Program DescriptionAnimal Care and Use Program

Division of Laboratory Animal Medicine

University of California, Los Angeles

10833 Le Conte Ave

Suite 16-222 CHS

Los Angeles, CA 90095March 30, 2017

ForAAALAC International

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Table of Contents

Section 1. Introduction...............................................................................................................1

Section 2. Description................................................................................................................7

I. Animal Care and Use Program...........................................................................................7

A. Program Management.....................................................................................................7

1. Program Management Responsibility............................................................................7

a. The Institutional Official..............................................................................................7

b. Role of the Attending Veterinarian..............................................................................7

c. Interinstitutional Collaborations.................................................................................11

2. Personnel Management..............................................................................................12

a. Training, Education, and Continuing Educational Opportunities...............................12

i. Veterinary and Other Professional Staff..............................................................12

ii. Animal Care Personnel.......................................................................................16

iii. The Research Team............................................................................................18

b. Occupational Health and Safety of Personnel..........................................................23

i. Institutional Oversight..........................................................................................23

ii. Standard Working Conditions and Baseline Precautions....................................28

1) Medical Evaluation and Preventive Medicine for Personnel................................28

2) Personnel Training Regarding Occupational Health and Safety.........................33

3) Personal Hygiene................................................................................................34

4) Standard Personnel Protection............................................................................35

iii. Animal Experimentation Involving Hazards.........................................................43

B. Program Oversight.........................................................................................................53

1. The Role of the IACUC/OB..........................................................................................53

a. IACUC/OB Composition and Function......................................................................53

b. Protocol Review........................................................................................................54

c. Special Considerations for IACUC/OB Review.........................................................58

i. Experimental and Humane Endpoints.................................................................58

ii. Unexpected Outcomes that Affect Animal Well-being.........................................60

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iii. Physical Restraint................................................................................................61

iv. Multiple Survival Surgical Procedures.................................................................62

v. Food and Fluid Regulation..................................................................................64

vi. Use of Non-Pharmaceutical-Grade Drugs and Other Substances......................64

vii. Field Investigations.............................................................................................65

viii. Animal Reuse.......................................................................................................65

2. Post-Approval Monitoring............................................................................................70

3. Investigating and Reporting Animal Welfare Concerns...............................................72

4. Disaster Planning and Emergency Preparedness.......................................................75

II. Animal Environment, Housing and Management..............................................................77

A. Animal Environment.......................................................................................................77

1. Temperature and Humidity..........................................................................................77

2. Ventilation and Air Quality...........................................................................................80

3. Life Support Systems for Aquatic Species..................................................................81

4. Noise and Vibration.....................................................................................................82

B. Animal Housing..............................................................................................................82

1. Primary Enclosures.....................................................................................................82

2. Environmental Enrichment, Social, and Behavioral Management...............................83

a. Environmental Enrichment........................................................................................83

b. Social Environment...................................................................................................84

c. Enrichment, Social and Behavioral Management Program Review..........................85

d. Procedural Habituation and Training of Animals.......................................................86

e. Sheltered or Outdoor Housing..................................................................................87

f. Naturalistic Environments.........................................................................................88

C. Animal Facility Management..........................................................................................88

1. Husbandry...................................................................................................................88

a. Food..........................................................................................................................88

b. Drinking Water..........................................................................................................95

c. Bedding and Nesting Materials.................................................................................96

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d. Miscellaneous Animal Care and Use Equipment......................................................97

e. Sanitation..................................................................................................................98

i. Bedding/Substrate Change.................................................................................98

ii. Cleaning and Disinfection of the Micro- and Macro-Environments....................100

f. Conventional Waste Disposal.................................................................................101

g. Pest Control............................................................................................................101

h. Weekend and Holiday Animal Care........................................................................102

2. Population Management............................................................................................103

a. Identification............................................................................................................103

b. Breeding, Genetics, and Nomenclature..................................................................104

III. Veterinary Care...............................................................................................................105

A. Animal Procurement and Transportation......................................................................105

1. Animal Procurement..................................................................................................105

2. Transportation of Animals..........................................................................................107

B. Preventive Medicine.....................................................................................................108

1. Animal Biosecurity.....................................................................................................108

2. Quarantine and Stabilization.....................................................................................110

3. Separation by Health Status and Species.................................................................114

C. Clinical Care and Management....................................................................................115

1. Surveillance, Diagnosis, Treatment and Control of Disease.....................................115

2. Emergency Care........................................................................................................121

3. Clinical Record Keeping............................................................................................121

4. Diagnostic Resources................................................................................................123

5. Drug Storage and Control..........................................................................................126

D. Surgery.........................................................................................................................127

1. Pre-Surgical Planning................................................................................................127

2. Surgical Facilities.......................................................................................................128

3. Surgical Procedures..................................................................................................129

4. Aseptic Technique.....................................................................................................130

5. Intraoperative Monitoring...........................................................................................133iii

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6. Postoperative Care....................................................................................................133

E. Pain and Distress.........................................................................................................134

F. Anesthesia and Analgesia............................................................................................136

G. Euthanasia...................................................................................................................138

IV. Physical Plant.................................................................................................................140

A. Facilities Overview.......................................................................................................140

B. Centralized (Centrally-Managed) Animal Facility(ies)..................................................141

C. Satellite Animal Housing Facilities...............................................................................158

D. Emergency Power and Life Support Systems..............................................................160

1. Power........................................................................................................................160

2. Other System Malfunctions.......................................................................................160

E. Other Facilities.............................................................................................................160

1. Other Animal Use Facilities.......................................................................................160

2. Other Animal Program Support Facilities..................................................................161

AppendicesAppendix 1: Glossary of Abbreviations and AcronymsAppendix 2: Summary of Animal Housing and Support SitesAppendix 3: Line DrawingsAppendix 3.1: Space UsageAppendix 4: Organizational Chart(s)Appendix 5: Animal UsageAppendix 6: Personnel Medical Evaluation FormAppendix 7: IACUC/OB Membership RosterAppendix 8: IACUC/OB MinutesAppendix 9: Blank IACUC/OB Protocol FormAppendix 10: IACUC/OB Periodic ReportAppendix 11: Heating, Ventilation and Air Conditioning (HVAC) System SummaryAppendix 12: Aquatic Systems Summary – Part I & IIAppendix 13: Primary Enclosures and Animal Space ProvisionsAppendix 14: Cleaning and Disinfection of the Micro- and Macro-EnvironmentAppendix 15: Facilities and Equipment for Sanitizing MaterialsAppendix 16: Lighting SummaryAppendix 17: Satellite Housing Facilities

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Appendix 18: ARC-approved Exceptions to Social Housing/Enrichment Appendix 19: Biological AgentsAppendix 20: Chemical AgentsAppendix 21: Animal Restraint DevicesAppendix 22: Multiple Major Survival SurgeriesAppendix 23: Food and Fluid RegulationAppendix 24: Surgical Facilities – DLAMAppendix 25: Surgical Facilities – PIAppendix 26: Drug ListAppendix 27: Euthanasia Locations (Study Areas)

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Program Description

Instructions for Completing and Submitting the Program Description for the Institutional Animal Care and Use Program

Section 1. Introduction

A. State the name of the program unit and, if applicable, its parent organization. List all organizations (schools, centers, etc.) included within the program unit.

Institution: University of California, Los Angeles.

Units comprising the accredited unit: 9*1) David Geffen School of Medicine2) School of Dentistry3) Jonathan and Karin Fielding School of Public Health4) College of Letters and Sciencea. Life Sciences Core Programb. Ecology and Evolutionary Biologyc. Microbiology, Immunology, & Molecular Genetics (MIMG)d. Molecular, Cell, and Developmental Biology (MCDB)e. Integrative Biology and Physiology (formerly: Physiological Sciences)f. Psychology5) School of Engineering and Applied Science (Department of Bioengineering)6) Brain Research Institute (BRI)7) Jules Stein Eye Institute (JSEI)8) Crump Institute of Biological Imaging (CIBI)9) Doheny Eye Institute (DEI)

*The first eight units do not have discrete corresponding vivarium locations. Rather, animals belonging to various units may be housed in a shared vivarium based on functional needs, e.g., imaging, breeding, behavioral testing. The ninth unit is located approximately 15 miles from the UCLA Campus.

B. Give a brief overview of the institution, its purpose and how the animal care and use program relates to the mission of the institution.

UCLA’s research program began in the early 1950s and today consistently ranks among the top universities with a research component. The UCLA campus, located on 419 acres in West Los Angeles, has a large teaching and research program with over 38,000 students. The level of UCLA’s research funding is approximately $1 billion in competitively awarded research grants and contracts in a single year (http://www.ucla.edu/research/). The two

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largest sources of research funding typically include the National Institutes of Health (NIH) and the National Science Foundation (NSF). Private donors and scientific foundations are also among UCLA’s chief supporters, accounting for as much as 20% of the research support budget. UCLA is firmly rooted in its land-grant mission of teaching, research and public service, which is reflected in the priorities of the animal care and use program as well.

C. Note that AAALAC International’s three primary standards are the Guide for the Care and Use of Laboratory Animals (Guide), NRC, 2011; the Guide for the Care and Use of Agricultural Animals in Research and Teaching (Ag Guide), FASS, 2010, and the European Convention for the Protection of Vertebrate Animals Used for Experimental and Other Scientific Purposes, Council of Europe (ETS 123). Other regulations and guidelines used (U.S. Department of Agriculture (USDA), Public Health Service (PHS) Policy, Good Laboratory Practice (GLP), Canadian Council on Animal Care (CCAC), etc.) may also apply. Describe which of the three primary standards and other regulations and guidelines are used as standards for the institutional animal care and use program and how they are applied. For example, an academic institution in the United States with an Office of Laboratory Animal Welfare (OLAW) Assurance may use the standards of the Guide and PHS Policy for all animals, the Animal Welfare Act regulations for covered species, and the Ag Guide for agricultural animals used in agricultural research and teaching (see also Guide, pp. 32-33). In the European Union, the standards applied might be the Guide, ETS 123, Directive 2010/63, and any country-specific regulations.

We follow the standards of the Guide and the PHS Policy for all vertebrate species, and the Animal Welfare Act regulations for USDA-covered species. Our program also includes a Good Laboratory Practice (GLP) component for the conduct of nonclinical studies (drugs, devices and biologicals) toward FDA submission.

D. Describe the organization and include an accurate, current, and detailed organizational chart or charts (see Appendix 4) detailing the lines of authority from the Institutional Official to the Attending Veterinarian, the Institutional Animal Care and Use Committee/Oversight Body (IACUC/OB), and the personnel providing animal care. Please include the title, name (Note: For individuals whose information is publically available, provide the titles and names; for individuals whose information is not publically available, you may provide titles only.), and degree (if applicable) of each individual at the level of supervisor or above. Names of animal care staff below the title of supervisor need not be included, but the titles and number of animal care personnel under each supervisor should be included. If animal care responsibility is administratively decentralized, including the management of satellite housing areas/locations, the organizational chart or charts must include all animal care programs, indicating the relationship between each administrative unit and personnel, the Attending Veterinarian, and the Institutional Official.

Organizational charts are included in Appendix 4.

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The Institutional Official (IO) also holds the title of Interim Vice Chancellor for Research (VCR) and reports to the UCLA Provost. The Attending Veterinarian (AV) directly reports to the IO on regulatory, accreditation and public relations matters. The VCR oversees the Office of Research Administration (ORA), which includes administrative support for the following:

Institutional Animal Care and Use Committee (IACUC), known at UCLA as the Animal Research Committee (ARC). The AV is a voting member.

Institutional Biosafety Committee (IBC). The AV designee is a voting member. Office of Contracts and Grants Administration (OCGA) and Extramural Fund

Management (EFM). No AV affiliation.

Additional units within the VCR organization include:

Technology Development Group (TDG). No AV affiliation. Research Policy and Compliance (RPC). No AV affiliation.

The Vice Dean for Research (VDR) of the School of Medicine reports to the Dean of the School of Medicine. He oversees the animal research program’s overall space allocation and, when necessary, financially supports the animal research operation. The AV directly reports to the VDR on financial support, per diem setting and facilities/equipment needs.

The AV (Campus Veterinarian) has direct and delegated responsibility for the animal research program. The AV is the Executive Director of DLAM and reports dually to the IO and the VDR. The AV directly supervises the following DLAM staff members: (1) Veterinarians (3 total); (2) Chief Administrative Officer; (3) Director of Operations; (4) Diagnostic Laboratory Manager, and (5) Chief Compliance Officer.The veterinarians oversee the veterinary technicians, clinical and surgical services, researcher training and compliance.

The Chief Administrative Officer administers the business and personnel side of the operation.

The Director of Operations oversees the animal resources managers and supervisors and, indirectly, the entire animal husbandry operation.

The Chief Compliance Officer acts as the QAU (Quality Assurance Unit) or QAU liaison for GLP studies, manages Standard Operating Procedures (SOPs) and oversees GLP archiving functions.

E. Identify the key institutional representatives (including, but not limited to, the Institutional Official; IACUC/OB Chairperson; Attending Veterinarian; animal program manager; individual(s) providing biosafety, chemical hazard, and radiation safety oversight; etc.); and individuals anticipated to participate in the site visit.

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IO: Ann R. Karagozian, PhD VDR: Stephen Smale, PhD IACUC (= ARC) Chair: Nigel Maidment, PhD AV and Director of DLAM: Jeffrey Goodwin, DVM, PhD, DACLAM RSAWA Director: Jennifer Perkins, MA, CPIA Assistant Vice Chancellor - EH&S: Colin Dimock, BA Biosafety, Chemical Hazard & Radiation Safety oversight:

o Biosafety Officer: Stacey Kraemer, PhD o Chemical Hygiene Officer: Scott Hsieh, PhDo Radiation Safety Officer: Bryan Ruiz

Medical Director, Occupational and Employee Health: T. Warner Hudson, MD FACOEM, FAAFP

Individuals listed above, and members of the RSAWA and DLAM supervisory, veterinary, and technical staff, will participate in the site visit as appropriate.

F. Briefly describe the major types of research, testing, and teaching programs involving animals and note the approximate number of principal investigators and protocols involving the use of animals. As mentioned in the instructions, please complete Appendix 5 (Animal Usage) or provide the information requested in a similar format as an Appendix.

As of December 2016, the number of Principal Investigators is 425 and the number of active protocols is 1,049. The primary areas of research are*:

ARC Report - Approved Protocols from the Prior MonthReport Period: 12/1/2016 - 12/31/2016

Department PIs ProtocolsANESTHESIOLOGY 7 19ANTHROPOLOGY 2 2BIOENGINEERING 4 8BIOLOGICAL CHEMISTRY 7 15BIOMEDICAL ENGINEERING 1 1CHEMICAL AND BIOMOLECULAR ENGINEERING 2 4CHEMICAL ENGINEERING 1 3CHEMISTRY AND BIOCHEMISTRY 4 9DEANS OFFICE-SCHOOL OF MEDICINE 1 1DENTISTRY 18 64DLAM 6 10ECOLOGY AND EVOLUTIONARY BIOLOGY 11 18ENVIRONMENTAL HEALTH SCIENCES 1 1HEAD & NECK SURGERY 9 19HEMATOLOGY-ONCOLOGY 1 3HUMAN GENETICS 6 13

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INSTITUTE FOR SOCIETY AND GENETICS 1 1INSTITUTE OF GENOMICS AND PROTEOMICS 1 2INTEGRATIVE BIOLOGY & PHYSIOLOGY 12 24LIFE SCIENCES CORE CURRICULUM 1 3MEDICINE-CARDIOLOGY 22 64MEDICINE-CENTER FOR HUMAN NUTRITION 1 1MEDICINE-DERMATOLOGY 1 2MEDICINE-DIVISION OF DIGESTIVE DISEASES 8 18MEDICINE-ENDOCRINOLOGY 1 3MEDICINE-ENDOCRINOLOGY 5 11MEDICINE-GASTROENTEROLOGY 6 12MEDICINE-GERIATRICS 1 2MEDICINE-HEMATOLOGY-ONCOLOGY 8 25MEDICINE-INFECTIOUS DISEASE 2 10MEDICINE-NANO MEDICINE 1 6MEDICINE-NEPHROLOGY 2 4MEDICINE-PULMONARY DISEASE 6 22MEDICINE-RHEUMATOLOGY 2 7MICROBIOLOGY, IMMUNOLOGY & MOLECULAR GENETICS (MIMG)

24 50

MOLECULAR & MEDICAL PHARMACOLOGY 17 37MOLECULAR CELL & DEVELOPMENTAL BIOLOGY

13 43

NEUROBIOLOGY 17 39NEUROLOGY 26 72NEUROSURGERY 6 16NURSING 2 2OBSTETRICS & GYNECOLOGY 6 9OPHTHALMOLOGY 17 31ORTHOPAEDIC SURGERY 9 20PATHOLOGY AND LABORATORY MEDICINE 16 37PEDIATRICS 16 31PHYSICS & ASTRONOMY 2 2PHYSIOLOGICAL SCIENCE 9 30PHYSIOLOGY 12 29PLASTIC SURGERY 1 8PSYCHIATRY AND BIOBEHAVIORAL SCIENCES 22 58PSYCHOLOGY 8 22PULMONARY AND CRITICAL CARE MEDICINE 1 2RADIATION ONCOLOGY 6 9RADIOLOGICAL SCIENCES 8 20SURGERY-GENERAL 7 14SURGERY-LIVER AND PANCREAS TRANSPLANT 5 20SURGERY-ONCOLOGY 2 4SURGERY-PEDIATRIC 1 11SURGERY-PLASTIC 1 4SURGERY-THORACIC 2 3

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UROLOGY 7 19TOTALS 425 1049

G. Note the source(s) of research funding (grants, contracts, etc.) involving the use of animals.

UCLA receives extramural funding from both federal and non-federal agencies, including state and local funds, private for-profit and non-profit entities. A list of funding agencies will be available for review at the time of the site visit, upon request.

H. List other units (divisions, institutes, areas, departments, colleges, etc.) of your organization that house and/or use animals that are not included in this Description. If any of these are contiguous, physically or operationally (e.g., same IACUC/OB, same animal care staff), with the applicant unit, describe the association. Explain why such units are not part of this program application.Note: Questions regarding this section should be forwarded to the AAALAC Office.

None. All Campus units are included in this Program Description.

I. Contract Facilities: If the institution contracts for animal care facilities or services for animals owned by the institution, the contractor and its AAALAC International accreditation status must be identified. If a contractor's animal care and use program is not accredited by AAALAC International, a brief description, following this Program Description outline, of the relevant contractor's programs and facilities must be provided. In addition, the species and approximate average number of animals housed in the contract facilities and the approximate distance between the institution's animal facility and the contract facility must be noted. Incorporation of the contractor program into the site visit schedule will be discussed with institutional representatives. If the institution does not contract for animal care facilities or services, so note.

UCLA currently does not contract for animal care services from another institution or facility.

J. Note other relevant background that will assist reviewers of this report.

None

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Section 2. Description

I. Animal Care and Use Program

A. Program Management

1. Program Management Responsibility [Guide, pp. 13-15]

a. The Institutional Official [Guide pp. 13-14]Describe how program needs are clearly and regularly communicated to the Institutional Official by the Attending Veterinarian, IACUC/OB, and others associated with the program.

The AV, ARC Chair, and RSAWA Director have a joint in-person meeting with the IO no less than quarterly to discuss animal research program needs; large scale program needs that impact other areas (e.g., safety) are brought to the Office of the Vice Chancellor for Research Safety Oversight Committee (OSOC), of which the IO and ARC Chair are members. The AV directly reports to and meets as frequently as needed with the IO and the VDR to provide and receive updates and to discuss the animal Program needs. The ARC submits semiannual inspection and program evaluation reports to the IO no less often than every six months (inspections are done on a rolling basis, so the reports go to the IO on a rolling basis as well). ARC meeting minutes are submitted to the IO upon approval, generally within a month of an ARC meeting. The AVC-EH&S has a dotted line to the IO regarding safety issues.

b. Role of the Attending Veterinarian [Guide, p. 14]

i. Describe the institutional arrangement for providing adequate veterinary care. Although individual name(s) and qualifications will be described below, identify by title the veterinarian(s) responsible for the veterinary care program, including: a list of responsibilities a description of the veterinarian’s involvement in monitoring the care

and use of laboratory animals the percentage of time devoted to supporting the animal care and use

program of the institution if full-time; or the frequency and duration of visits if employed part-time or as a consultant.Note: If preferred, this information may be provided in a Table or additional Appendix.

UCLA employs 4 full time veterinarians devoted (100% time) to supporting the animal care Program. Veterinarian Title

Responsibilities/laboratory animal monitoring involvement

% time

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Attending Veterinarian (AV) and DLAM Exec. Director

Serves on the ARC; is the Executive Director of the Department of Laboratory Animal Medicine (DLAM); in collaboration with theVivarium Operations Director, establishes the methods and procedures for the housing, feeding, care and use of all research animals housed at UCLA facilities, and ensures that adequate veterinary care is provided to all animals used in research, teaching and testing; authorized to enter any place within the jurisdiction of UCLA to conduct on-site inspections of animal facilities and animals to ensure that husbandry practices and animal health and research techniques are in compliance with relevant federal, state, local and institutional requirements; authorized to halt any animal activity if the safety or welfare of an animal is at risk or if the work being performed on a project is not in accordance with the approved protocol; directs the service arm of the animal Program, including budgetary considerations involving animal care, strategic planning and the approval of animal facility renovations and new construction

100

Clinical Veterinarian, Research Support

Serves as an alternate member on the ARC; conducts ARC protocol veterinary pre-reviews; assists the AV in carrying out all of the responsibilities of the AV role especially in regard to USDA covered species researcher support, compliance, and technical service; oversees the researcher training program, and surgical and technical services for all species including the pharmacy; investigates and coordinates with the ARC regarding animal research compliance issues mostly involving USDA-covered species; assists researchers with model and procedure development mostly involving USDA-covered species.

100

Clinical Veterinarian, Pre-clinical and Regulatory Affairs

Serves on the ARC and IBC; conducts ARC protocol veterinary pre-reviews; assists the AV in carrying out all the responsibilities of the AV role especially in regard to rodent researcher support and compliance; serves as Study Director/SD liaison for GLP studies involving rodents; oversees the program of weekly animal care and compliance visits to all study areas on campus, investigates and coordinates with the ARC regarding animal research compliance issues mostly involving rodents; assists researchers with

100

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model and procedure development mostly involving rodents. Conducts ARC veterinary protocol pre-reviews, primarily rodent-based protocols and procedural amendments.

Clinical Veterinarian, Colony Health

Conducts ARC protocol veterinary pre-reviews; assists the AV in carrying out all of the responsibilities of the AV role especially in regard to rodent and USDA-covered species clinical care; manages the programs for rodent health, USDA-covered species health, environmental enrichment, and rodent sentinels.

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ii. List others (e.g., Principal Investigators, veterinarians serving as Principal Investigators, veterinary faculty/staff, technical staff, farm managers) who have a direct role in the provision of veterinary care and describe their responsibilities. The Organizational Chart(s) provided in Appendix 4 must depict the reporting relationship between these individuals and the Attending Veterinarian.Note: If preferred, this information may be provided in a Table or additional Appendix.

Position Title ResponsibilitiesAnimal Resources Supervisor/Import Coordinator

Supervise the Rodent Health Team – 4 direct reports; 6 indirect reports. Schedule and conduct rodent health rounds, administer treatments when necessary, Monitor active health cases through the REACTOR program.

Animal Health Technician III (Surgery and Anesthesia)

Manages USDA-covered species surgery core providing support in anesthesia, surgery, and non-surgical procedures as well as health rounds for different covered species. Provides pre and post-operative care / treatments (covered species). Provides anesthesia support for non-surgical procedures (MRI, CT scans, Fluoroscopy, PET Scans, X rays) at different locations.

Animal Health Technician IV (Rodent Health/Technical Services)

Teaches rodent health to newly assigned health technicians. Provides technical support for the DLAM Technical Services including tail vein injections, gavage, blood collection, tissue harvesting. Maintains the rodent surgery room by scheduling and cleaning for the investigators. Provides support in animal health, including

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proper assessment and treatment of the abnormal conditions in mice, rats, and birds. Provides limited administrative assistance with REACTOR and email contact lists for communication with investigators. Assists lab members with hands-on training and assistance with regards to properly administrating medication and performing minor procedures.

Animal Health Technician III (Study Areas)

Manages and performs weekly rounds of all study areas, which includes animal health checks and compliance.

Animal Health Technician III (Surgery and Anesthesia)

Manages USDA-covered species surgery core providing support in anesthesia, surgery, and non-surgical procedures as well as health rounds for different species. Manages controlled substances supply. Provides NHP training and covered species aseptic training. Supports environmental enrichment team.

Animal Health Technician IV/Environmental Enrichment Coordinator

Environmental Enrichment and Behavioral Management program development and oversight, animal health rounds for various species, technical services, rodent surgery, assisted reproductive technologies in mice and serves as an instructor for on-site lab animal workshops for veterinary technology colleges.

Animal Health Technician Provides support in anesthesia, surgery, and non-surgical procedures, maintains medical records in USDA covered species. Health rounds for different non USDA-covered species including but not limited to rodents.

Animal Technician (Rodent Health/Technical Services)

Reports rodent health cases and monitors condition and treatment of sick animals. Communicates with labs via REACTOR and updates case records daily. Staffs DLAM pharmacy and processes orders for labs. Performs technical services and treatments for labs if requested.

Staff Research Associate II (Rodent Health/Technical Services)

Rodent health team member: daily response, assessment, and treatment of mice in multiple rodent barriers. Under

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veterinarian guidance evaluates cases, inputs/update health program database, communicates with investigators, and follows up to case resolution. Technical services team member: Supports research requests - provides dosing and tissue collection in rodent species. Well-versed in various delivery techniques in rodents.

Animal Technician (Enrichment) Provides daily enrichment to all species.

Staff Research Associate/Training and Technical Services Manager

Teaches mouse, rat, aseptic technique, and other species-specific classes, as well as surgical and non-surgical techniques requested by investigators. Provides support in anesthesia, surgery, and non-surgical procedures as well as health rounds for different species. Manages the colony of mice and rats used for training.

Staff Research Associate II/Training Technician

Teaches mouse, rat, aseptic technique, and other species-specific classes. Provides support in surgical and non-surgical procedures as well as rodent health rounds when necessary.

Assistant Animal Technician/Training Technician

Assists the Training Manager and the Training Technician in all the activities associated with hands on classes including animal handling.

All other Animal Care Staff Daily cage observations and animal health checks; senior animal care staff may provide more detailed animal (health case) observation and administer topical, oral, and injectable medications or other health treatments under the direction of a veterinarian

Principal Investigator and/or Research Staff

Provide animal (health case) observation and administer topical, oral, and/or injectable medications or other health treatments under the direction of the veterinary staff

c. Interinstitutional Collaborations [Guide, p. 15]Describe processes for assigning animal care and use responsibility, animal ownership and IACUC/OB oversight responsibilities at off-site locations for interinstitutional collaborations.

For UCLA-sponsored research conducted off-site, the ARC requires the PI to submit a 11

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copy of the protocol and approval notice covering animal activities at the offsite location, with the exception of work conducted at the VA Greater Los Angeles Healthcare System, which is covered by a Memorandum of Understanding (MOU) that details reviewing and reporting responsibilities of each IACUC. Research performed with animals in field settings requires ARC review on UCLA forms.

2. Personnel Management

a. Training, Education, and Continuing Educational OpportunitiesDescribe how the IACUC/OB provides oversight and evaluates the effectiveness of training programs and the assessment of personnel competencies. Describe how training is documented.Note: Do not include details about the training program, which should be described in the following sections.

The ARC has established minimum requirements for participation in animal research activities and ties completion of these requirements to protocol approval. Each person that will handle live animals must complete (i) online regulatory training via the Collaborative Institutional Training Initiative (CITI) program, and (ii) species-specific training through either DLAM or a certified in-lab trainer (especially when species-specific training is best provided by investigators more closely familiar with non-traditional species, such as bats).

The ARC administrative staff within RSAWA is responsible for updating CITI and species-specific training completion in the online Research Application Tracking System (RATS) database. The ARC administrative staff also records completion of aseptic surgical techniques training through DLAM and annual participation in the occupational health program.

Effectiveness of training is checked ad hoc on a risk-based, case-by-case basis, e.g., proficiency in euthanasia by physical method is verified by DLAM trainers or the ARC Animal Welfare Administrator at the time of first occurrence after training has been delivered. Also, the ARC codicil mechanism is used in some cases to assure that, e.g. a complicated or potentially painful procedure is being performed correctly by a researcher with documented training. The effectiveness of the training program is also evaluated as part of the post-approval monitoring program which includes the ARC semiannual program review and inspections.

i. Veterinary and Other Professional Staff [Guide, pp. 15-16]For the Attending Veterinarian and other individuals having a direct role in providing veterinary medical care (veterinarians, other professional staff listed above, private practitioners, etc.), provide: name, credentials (including degrees), and a description of their qualifications, training, and continuing education opportunities.

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Note: Please do not provide curriculum vitae of personnel; if preferred, this information may be presented in a Table or additional Appendix.

Veterinarian/Professional Staff Name

Credentials, Qualifications and Training

Jeffrey Goodwin DVM(1993), PhD(1996), DACLAM(2003). USDA Accredited.Laboratory Animal Veterinarian since 1997. Member of national AALAS, ASLAP, AVMA, Society for Quality Assurance. Attends local and national meetings regularly

Sandra Duarte-Vogel DVM (2004), DACLAM (2011). USDA Accredited.14 years of experience in laboratory animals in academic and industry environments, LAM resident at UCLA. Member of local and national AALAS, APV, CLAMS, AVMA, and ACLAM exam committee. Attends local and national meetings on the regular basis.

Joanne Zahorsky-Reeves DVM (1995), PhD (1999), DACLAM (2011)13 years NIH-funded research in lab animals, 10 years private practice (part-time / relief), and 12 years full-time lab animal experience. Cornell Vet graduate. PhD in Comp and Exp Medicine, U Tennessee. Post-doc in xenotransplantation, Keck School of Medicine, USC. Member of AALAS, AVMA, ACLAM, Amer Coll of Toxicology, CLAMS; USDA-accredited and CA-state licensed. Attends national and regional meetings (ACLAM Forum, AVMA, AALAS, Society for Quality Assurance).

Cris Torres DVM, MPH, Clinical Veterinarian, USDA Accredited, licensed to practice medicine in Texas and California. 25 years of animal experience, 11 years with lab animals. Member of AVMA, AALAS, APV, and VECCS. Attend annual symposiums, leadership meetings and social events, attend webinars and seminars offered through National AALAS and other Veterinary organizations.

In general, for the DLAM veterinary staff below, all receive one-on-one training from the veterinarians, supervisors, training specialists, Chief Compliance Officer and EH&S staff in University and DLAM policy and procedures, performing animal health inspections, regulatory issues, and safety. Veterinary technicians receive species-specific training for restraint, phlebotomy and other techniques.

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Linda Robertson AS, BS, RVT, LATg, CMARNational AALAS Member, Treasurer, Southern California Branch – AALAS. Plan and coordinate continuing education opportunities for SCB AALAS membership through. Attend annual symposiums, leadership meetings and social events, attend webinars and seminars offered through National AALAS

Guillermo Moreno BS, RVT, LATOver 11 years of lab animal experience, over 15 years of small animal veterinary medicine experience (Emergency and General practice). Member of SCB-AALAS, National AALAS, EVCCS, Anesthesia Nerds.

Carmen Volpe BA, AAS, RVT, LATG12.5 years of lab animal experience (including 4 years in training, 5 years as supervisor, and 3 years focused on rodent health), 4 years of small animal practice, 2 years of animal shelter medicine, 2 years of teaching the Veterinary Assistant program at Apollo College. Attends local and national AALAS meetings. Member of AALAS, SCB-AALAS.

Alex Lo RVT, RLATG, BSMember of SLAVT. 13 years of laboratory animal experience. Attended AALAS National meetings, ASEC Symposiums, UCI Conti Symposiums, SCVMA veterinary Conti Symposiums, SCBAALAS Lab Animal Symposiums, Cal Poly Pomona Summer Symposiums, Western Veterinary Conference, AALAS Behavioral Management of Nonhuman Primates in Research Colonies Webinar, AALAS learning library.

Renee Hlavka Lock AS, BS, RVT, LATG7 years’ lab animal experience. Member of AALAS and ASR.

Anastasia Schimmel BS, RVT, RLATG12.5 years of laboratory animal experience, holds memberships in SCB-AALAS and National AALAS. Attends local and national AALAS meetings and continuing education courses in veterinary technology.

Adriana L. Gallardo RVT, LATG8 years of lab animal experience at UCLA, 2 years of shelter medicine experience, 3 years’ small animal practice experience. Member of

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SCB-AALAS, National AALAS. Has attended local and national AALAS meetings.

Mary Loutzenhiser BS, LATG6 years of experience in laboratory animals as Animal Technician at UCLA/DLAM. 3 years of experience on UCLA DLAM hazard containment husbandry team. Member of SCB-AALAS and National AALAS.

Tim March BS, LATG18 years of lab animal experience. Attends local and national AALAS meetings.

Ruben Angeles BS, LATG11 Years animal lab experience. Attended Symposium on Social Housing of Laboratory Animals in March 2016

Andrea Knipe BS, RVT, LATG10 years of lab animal experience, 4 years of small animal practice experience. Attends local and national AALAS meetings. Member of AALAS, SLAVT, LAWTE, ASR. Serves on the IACUC for Platt College Ontario/Riverside and Pierce College and actively volunteers for LAWTE and SLAVT.

Heather Troupe AS in Animal Science/Veterinary Technology, ALAT certified5 years of experience in private practice. 5 year of experience in laboratory animals at UCLA/DLAM, including breeding colony management and training. Member of SCB-AALAS, National AALAS. Has attended locals and national AALAS meetings.

Alma Silva 4 years of experience in laboratory animals as Assistant Animal Technician and training technician at UCLA/DLAM. Member of SCB-AALAS and National AALAS

During the past three years, DLAM has supported the veterinarians and veterinary staff to attend a variety of continuing education courses including, but not limited to: AALAS local branch seminars, workshops, training symposium (SCB-

AALAS/Palms to Pines) AALAS Learning Library On-line Courses AALAS National Meetings including workshops Academy of Surgical Research National Meeting ACLAM Forum

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Association of Primate Veterinarians Charles Louis Davis, D.V.M. Foundation Continuing education courses offered by campus Human Resources National Society for Histotechnology Conference Newco Distributors Open House in Rancho Cucamonga, California Primate Training and Enrichment Workshop Swine Cannulation Workshop at University of CA, Irvine Society of Quality Assurance (SQA) Scientists Center for Animal Welfare (SCAW) Symposium on Social Housing of Laboratory Animals UC System-wide Vet Director’s/IACUC meeting Vet Med Team On-line Courses Webinars hosted by various organizations and regulators (ie. NABR, VBI)

ii. Animal Care Personnel [Guide, p. 16]

1) Indicate the number of animal care personnel.

There are 94 members of the DLAM animal care staff (excluding veterinary staff captured in section 1.A.2.a.i.), including: 1 Lab Helper 31 Assistant Animal Technicians 32 Animal Technicians 7 Staff Research Associates 14 Senior Animal Technicians 4 Principal Animal Technicians 2 Animal Resources Supervisors 3 Animal Resources Managers.

2) Summarize their training, certification level and type, experience, and continuing education opportunities provided.Note: If preferred, this information may be provided in a Table or additional Appendix.

Animal Cares Staff Certification Summary: 02 = CMAR 15 = LATG level 09 = LAT level 19 = ALAT level

Summary of training, experience and continuing education opportunities:Laboratory animal work experience for all animal care staff ranges from at least 1 to 31 years at UCLA alone.

In general, DLAM personnel receive training on all aspects of laboratory 16

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animal care, including safety and University and Departmental policies. Training is provided by Animal Resource Supervisors/Managers and Senior/Principal Animal Technicians and Veterinarians as well as Environmental Health & Safety staff.

All new husbandry technicians receive a minimum of 2 weeks basic training in animal handling and vivarium procedures and policies (primarily with rodents). The trainer continues to work with the trainee for 2 additional weeks before completing the training, usually in 4 weeks. Cross training to expose the technician to other species or facilities takes place after the employee successfully passes the 6-month employment probationary period. At this time, the employee will also be considered for the weekend/holiday rotation.

All personnel (including lab and hazardous containment technicians), working within vivaria, complete or attend the following training classes conducted by Environmental Health and Safety at required time intervals: Laboratory Safety Fundamentals (annually) Medical Waste Management (select staff; every 3yrs) Blood borne Pathogens (annually) Respirator fit training and testing (annually)

All personnel working within hazardous containment vivarium complete or attend the following training classes conducted by Environmental Health and Safety or AALAS at required time intervals: Biological Safety Cabinets (every 3yrs) Biosafety A, B, C's--Biosafety Level 2 (every 3yrs) Biosafety Level 2+(every 3yrs)

Select personnel, working with NHPs and/or tissues, attend the following training at required time intervals: B virus exposure training (annually)

Select diagnostic lab personnel attend and maintain certification for trainingclasses conducted by Environmental Health and Safety: Shipping Biologicals

Monthly all-staff meetings are held to discuss UCLA/Departmental issues, and a significant portion of the meeting is devoted to education and training. Topics include, but are not limited to safety, zoonoses, ergonomics, animal health issues, biohazardous/chemical spill training, regulatory updates, as well as research topics presented by guest Principal Investigators. Supervisors and Managers conduct at least monthly group meetings with staff; SOP and other training is a regular component of these meetings.

GLP training is provided at least annually and in preparation for studies aimed

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at receiving FDA approval.

In addition, upon request or when a general need has been identified, AALAS certification courses (led by Veterinarians, Supervisors, Principal Animal Technicians and Managers) are provided weekly throughout the year to review study materials and questions.

Continuing education, AALAS certification and ongoing registry are highly encouraged. Promotions and incentive awards are based in great part on AALAS certification. Each year, selected staff members are sent to the local, regional and National AALAS meetings, and other relevant programs throughout the year for continuing education. During the past three years, DLAM has supported animal care staff to attend the following continuing education courses including, but not limited to: AALAS local branch seminars, workshops, training symposium (SCB-

AALAS/Palms to Pines AALAS) AALAS Learning Library On-line Courses AALAS National Meetings including workshops Continuing education courses offered by campus Human Resources Newco Distributors Open House in Rancho Cucamonga, California Vet Med Team On-Line Courses Webinars hosted by various organizations and regulators (ie. NABR, VBI)

All training records will be available for review at the time of the site visit, upon request.

iii. The Research Team [Guide, pp. 16-17; 115-116; 122; 124]

1) Describe the general mechanisms by which the institution or IACUC/OB ensures that research personnel have the necessary knowledge and expertise in the animal procedures proposed and the species used.

The ARC mandates that all Principal Investigators, as well as all personnel having direct contact with live vertebrate animals (this includes investigators, instructors, technical staff, trainees, students, husbandry and visiting personnel), must have relevant training and/or experience with the animal procedure(s) and the animal models used prior to initiating work with laboratory animals. The ARC and DLAM work together to ensure this. To that end, a detailed description of qualifications and relevant experience and/or a training plan, is provided in the research protocol. At the time of protocol submission, ARC staff determine, and relay to the PI, the additional training needs of each person listed on the protocol needed to secure protocol approval. This determination is based on whether the following three basic required components have been completed:

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1. An online tutorial covering basic animal welfare andIACUC subjects (‘Working with the IACUC’; CITI)2. Other relevant online training modules, such as:

a. Aseptic Surgery (CITI)b. Post-Procedure Care of Mice and Rats in Research: Minimizing Pain and Distress (CITI)c. Species-Specific Training (amphibians, mice, rats, hamsters, gerbils, guinea pigs, rabbits, dogs, swine, NHP, zebrafish; CITI)

3. Hands-on Species-Specific Training (hands on animal handling and euthanasia conducted by DLAM staff or certified in-lab trainer for most species and by PI for fish, reptiles, bats, birds and amphibians other than frogs)

Documentation of completion of CITI courses is available to ARC staff on the CITI website. ARC staff also receive daily completion reports from CITI. Training documentation reflecting completion of hands-on training is submitted (by DLAM or in-lab certified trainers) to the ARC, who maintains the database of trained animal researchers. Again, ARC staff will not issue approval for any application unless they have documentation showing that all personnel listed on the protocol have completed the above training, as appropriate. Training specific to research procedures, including specific surgical techniques, sample collection, substance administration and tissue harvesting are generally provided by the PI/in lab trainer but are also offered by DLAM. Documentation of this training may be reviewed as part of the Post-Approval Monitoring (e.g. ARC inspections) programs. Finally, prior to research personnel receiving access to the animal facility, DLAM staff verify that the applicant is listed on an approved protocol (and thus current on the above training) and has completed the following (as applicable):

1. Relevant online training modules:a. Working in the Animal Facility (DLAM)b. Hazard Containment (DLAM)2. A walkthrough and orientation for the applicable animal facility.

a) Briefly describe the content of any required training.

In addition to the online CITI modules mentioned above, the ARC mandates hands-on classes for species-specific training as well as aseptic technique. Species-specific Training classes include: Identification of abnormal conditions, including those that are

associated with pain and distress Emergency contact information Species normal behavior Safe handling and restraint

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Animal monitoring during restraint Hazardous and occupational health risk, including animal bites, and

how to proceed if exposure happens Euthanasia How to obtain additional training

Aseptic Technique class includes: Surgery suite and prep room set up How to operate equipment including anesthetic machine, heat source

and glass bead sterilizers Preemptive pain medications, anesthesia induction, maintenance and

monitoring How to prepare an animal aseptically for surgery Surgeons attire, hand scrub, and sterile gloves Sterile instruments and the surgical field Recovery from anesthesia, and post-operative care

DLAM-provided online courses (required for entry to the animal facilities) and content are as follows:Working in a Barrier Facility DLAM Facility Introduction/Definition of a Barrier Entering a Barrier Facility Personal Protective Equipment (PPE) Lab Equipment and Supplies Hand Cart Usage Biological Safety Cabinets (Setup, Usage, Cleanup) Animal Care (Handling, Requests, Returns, and Transfers) Clean/Used Cart Storage Sentinel Cages Rodent Room Classification System Procedure Rooms Euthanasia Exiting the Barrier

Hazard Containment Introduction to Hazard Containment Requirements Entering a Hazard Containment Facility Inside the Hazard Containment Facility Hazard Signage Personal Protective Equipment (PPE) Lab Equipment and Supplies Biological Safety Cabinets (Setup, Usage, Cleanup) Animal Care (Cage Usage, Identification, Transfers) Euthanasia

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Hazardous Waste disposal De-Gowning Procedures

b) Describe the timing of training requirements relative to the commencement of work.

All required training (see answer to question in section 2.2.a.iii.1 for required training list) must be completed prior to commencement of work with animals. ARC protocols are not approved until training is completed. Security access to the animal facility is not granted until individuals are listed on an approved ARC protocol.

c) Describe continuing education opportunities offered.

Ongoing educational needs are assessed at the time of protocol review (e.g. initial, renewal, amendment submission), and during for-cause compliance or PAM visits. ARC and DLAM staff are available to provide consultation and assistance to research personnel in areas such as ARC policies and guidelines, protocol writing/pre-review services, performance and documentation of searches for alternatives to the use of animals, unnecessary duplication and avoidance or minimization of painful or distressful procedures. DLAM staff is available for one-on-one training for specialized techniques as requested. DLAM staff is available to assist during model development or for the implementation of new protocols.

2) Describe the process(es) to ensure surgical and related procedures are performed by qualified and trained personnel, including: who determines that personnel are qualified and trained for surgical

procedures the roles that the Attending Veterinarian and IACUC/OB have in

this determination [Guide, pp. 115-116]

The ARC mandates that all personnel performing surgery and related procedures must have relevant training and/or experience with these procedure(s) prior to initiating that work with laboratory animals. The ARC/DLAM work together to ensure this.

A detailed description of qualifications, or a training plan, is provided in the research protocol. All new/renewal animal use protocols with USDA pain category D and E procedures are reviewed by a veterinarian prior to consideration by the Committee, and surgical preparation and techniques are reviewed at this time. At the time of protocol submission, ARC staff determine and relay to the PI the additional training needs of each person listed on the protocol. In the absence of training/experience, the ARC may require training through DLAM and/or veterinary oversight and verification of proficiency.

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Research staff beginning their animal work at UCLA are required to take the Aseptic Surgical Techniques online and/or lecture (prerequisite) followed by the wet lab class (taught by dedicated DLAM trainers) before performing survival surgery on any warm blooded vertebrates as described in the protocol. Successful completion of the online module is required before personnel are allowed to enroll in and attend the in-person session. Both portions of the training must be completed prior to being certified to perform survival surgeries. Individuals performing survival surgical procedures on covered species are monitored by qualified DLAM staff to ensure appropriate technique is employed. When new surgery protocols are initiated on USDA-covered species, a DLAM veterinarian will be present during the first few surgeries if instructed by the ARC, or if the PI has requested assistance. In addition, it is common for the ARC to ask a researcher to work with a DLAM veterinarian when performing a surgical procedure new to the lab, regardless of species. The language for this request for post-approval oversight is included in a codicil on the ARC approval notice. Codicils are agreements between the ARC and PI regarding some action that is required related to the protocol. For example, when a veterinary training or oversight codicil is placed on an approval notice, the codicil must be fulfilled before staff are allowed to work independently.

3) Describe the training and experience required to perform anesthesia. [Guide, p. 122]

During the aseptic surgical techniques course, assessing an adequate plane of surgical anesthesia, monitoring of vital signs during anesthesia, proper thermal and fluid support, and recovery from anesthesia are discussed and demonstrated by the dedicated DLAM trainers. Anesthetic choice and dose are discussed with investigators during veterinary pre-review of animal use protocols. In general, use of inhalation anesthesia is recommended over that of injectable regimens. Training in the use of isoflurane vaporizers is provided by DLAM. Investigators using USDA-covered species meet with a DLAM veterinarian to discuss the proposed use of anesthetics and analgesics in the animal use protocol. Most survival surgeries in USDA-covered species are coordinated (e.g. anesthesia performed) by DLAM (or TRIC) technicians with close veterinary oversight. For those surgeries where a DLAM veterinarian is not regularly involved, a veterinarian may be required to be present during the first few surgeries to ensure that anesthesia and monitoring are adequate for the procedure (this would be specified in a codicil to the approved protocol).

4) Describe how the proficiency of personnel conducting euthanasia is ensured (especially physical methods of euthanasia). [Guide, p. 124]

DLAM provides information on appropriate methods of euthanasia for any 22

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given species in the species-specific training classes. Rodent users receive information on euthanasia techniques during the didactic portion of the training class, and information is provided in the online handouts as to what methods are acceptable, and how they should be performed. Acceptable methods of euthanasia are covered during online species-specific training for each species, and also reemphasized during barrier walkthrough orientations. Trainees are instructed to ascertain death prior to disposal. Euthanasia techniques are also discussed with investigators during the veterinary pre-review of ARC protocols. Individual investigators are responsible for training lab personnel in the use of ARC-approved physical euthanasia methods, and for ensuring that guillotine blades are kept in good condition if this method is employed. For investigators requesting euthanasia without use of anesthetics, the ARC will routinely place codicils requiring verification of proficiency for personnel conducting physical methods on conscious animals.

b. Occupational Health and Safety of Personnel [Guide, pp. 17-23]

i. Institutional Oversight [Guide, pp. 17-19]

1) List the institutional entities (units, departments, personnel, etc.) that are involved in the planning, oversight, and operation of the institutional occupational health and safety program related to animal care and use (e.g., office(s) of environmental health, institutional health services or clinics (including contracted health services), industrial hygienists, Institutional Biosafety Committee(s) and/or Officer(s), Radiation Safety Committee(s) and/or Officer(s).

• Include a brief description of their responsibilities and qualifications.• If contracted services are used, also include their location (e.g.,remote

offices to which personnel must report).

The UCLA laboratory animal occupational health and safety (OHS) program is the responsibility and result of the coordinated efforts of several offices:

Planning: Hazard identification and risk assessment are done between DLAM, EH&S and the OHS Medical Director, Occupational and Employee Health. Input is also provided by ARC and IBC members experts, during protocol review, and the OHSCC (see below under Coordination).

Oversight: DLAM animal care staff control access to the centralized animal facility by DLAM and research staff and are available to escort visiting research or other personnel (e.g. Facilities workers) into these animal facility areas, as needed. Some oversight (e.g. compliance with Occ. Health directives) is also exerted by EH&S, the IBC, and the ARC during their routine or directed inspections and during ARC and IBC

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protocol review. Operation: This is the exclusive responsibility of the OHS facility

professionals. Coordination: The Occupational Health and Safety Coordinating Council

(OHSCC) was launched in 2010 to improve coordination between the different units on campus that deal with issues associated with human health and safety of researchers and staff working with animals. The OHSCC also discusses issues related to the protection of research animals in the context of exposure to human workers and zoonosis. OHSCC membership includes leadership/directors of Environment, Health & Safety (EH&S), Office of the Vice Chancellor for Research (OVCR), Occupational Health Facility (OHF), Research Safety & Animal Welfare Administration (RSAWA), and Division of Laboratory Animal Medicine (DLAM). The OHSCC advises the VCR and, where necessary, recommends policies on issues related to health and safety of personnel working with or near laboratory animals, as well as related to safety of animal subjects when zoonosis is a concern.

Key Animal OHSP Staff Qualifications/ResponsibilitiesT. Warner Hudson MD (1976), FACOEM (1994),

FAAFP (1979). Medical Director, Occupational and Employee Health; IBC and OHSCC member

Colin Dimock CHP(). AVC – EH&S, OHSCC member

Stacey Kraemer PhD (1996), RBP (2009), CBSP (2010). UCLA Biosafety Officer, IBC member, OHSCC Member

Bryan Ruiz CHP (2013). UCLA Radiation Safety Officer, RSC member

Matt Damron UCLA Laser Safety OfficerScott Hsieh PhD (1993). UCLA Chemical

Hygiene Officer, Chemical and Physical Safety Committee member

Jeffrey Goodwin DVM (1993), PhD (1996), DACLAM (2003). Lab animal vet since 1997. Ex. Director of DLAM. Serves on ARC, OHSCC.

Martha Maxwell BS (2001), CMAR (2010). Lab animal care since 1998. Animal Resource Manager. Hazard Containment and Dept. Safety Officer, DLAM. Attends IBC, OHSCC meetings. Coordinates DLAM safety program including

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IIPP meetings and hazardous agent training and Safety Considerations meetings with researchers.

Nancy Wayne PhD (1988). AVC – Laboratory Safety and Chair OHSCC.

Nigel Maidment PhD (1989). ARC ChairSamson Chow PhD (1983). IBC Chair, ESCRO

committee memberRSAWA Staff ARC and IBC administrative

staff coordinate with EH&S subject matter experts and relevant compliance committees

2) Describe methods to identify work-related hazards and the processes used to evaluate the significance of those hazards in the context of duties and tasks. Describe both common approaches and differences, if applicable, for categories of personnel such as, but not limited to, researchers, veterinarians, husbandry staff, cage-washing staff, students, housekeeping, physical plant staff, security personnel, IACUC/OB members (including non-affiliated members), contractors, visitors, etc. [Guide, pp. 18-19; see also Chapters 2 and 3 in Occupational Health and Safety in the Care and Use of Research Animals, NRC 1997.].

The Institution provides an occupational health and safety program that is consistent with federal, state and local regulations. All personnel involved in the care and use of research animals, including those in DLAM, investigator staff/students, personnel that handle animal tissues, and all PIs and faculty sponsors of ARC protocols (regardless of whether they handle animals), must be enrolled in the program. UCLA Policy 990, “Use of Laboratory Animal Subjects in Research,” describes the requirement for annual submission of the Medical History Questionnaire (MHQ) for review by Occupational Health Facility (OHF) personnel. The MHQ assists the OHF personnel to identify general lab animal or animal facility related hazards in the context of an individual’s exposure risks. In the context of protocol review, the ARC notifies individuals whose MHQs are expired or about to expire and will hold approval until MHQs are filed.

For research related hazards, ARC and IBC administrative staff coordinate with EH&S subject matter experts and relevant compliance committees to ensure that appropriate reviews and approvals are in place or under way prior to ARC approval. Specifically, during ARC protocol review, the PIs are asked to identify anticipated use of hazardous materials (e.g., chemical, biological, radiologicals), or the use of equipment which produce hazardous atmospheres (ionizing or non-ionizing radiation-producing devices, those which may impact air quality). These ARC protocols are referred to the appropriate

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subject matter experts to ensure that the procedures and conditions for safe handling of these materials/equipment have been reviewed by the relevant safety committee (e.g., IBC, RSC) and/or EH&S subject matter expert (e.g., chemical hygiene officer, laser safety officer, industrial hygienist) to ensure personnel and environmental safety plans are in place to maintain human and environmental health and safety standards.

DLAM and EH&S work together to ensure that all other visitors to the animal facility, such as facility maintenance or support workers and contractors not captured as personnel on an ARC or other research or safety committee protocol, receive training appropriate to their assigned task in the animal facility. At a minimum, this would include General Awareness Training, provided by DLAM, which includes a discussion of the general hazards found in animal facilities. DLAM will not issue or approve access to the DLAM animal facility until appropriate training (and in some cases, additional requirements such as enrollment in the MHQ program, vaccinations, TB testing, etc.) has been provided. Facilities personnel are trained to contact DLAM before entering any area where animals are present and are encouraged to contact EH&S with concerns or questions about any area where they may be unsure of the risks.

3) Describe methods and frequency of reassessing work-related hazards.

Risks associated with various biohazardous agents and related activities are evaluated in the context of the IBC risk assessment on a triennial basis or when new activities are proposed that affects the risk assessment.

Risks associated with other hazards found on an ARC protocol are referred to the appropriate EH&S subject matter expert for evaluation, similar to the IBC assessment.

All animal users complete the Medical History Questionnaire (MHQ) on an annual basis and this provides a preliminary evaluation of personal health risks as they relate to all work-related hazards. ARC approval is not granted for protocols that have personnel with expired MHQs. Personnel are encouraged to self-declare any changes in personal health risk for consultation through OHF when these issues arise.

4) Describe institutional programs or methods used to track and evaluate safety-related workplace incidents, including injuries, exposures, accidents, etc. Include the frequency of such assessments. [Guide, pp. 18-19]

There are several mechanisms by which safety-related workplace incidents and injuries are reported, investigated and corrected:

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All UCLA research personnel have been trained (through required EH&S training) to report all serious injuries to a 24/7 UCLA reporting hotline for immediate reporting, investigation and corrective action planning (as per Cal-OSHA requirements). The requirement and procedure are reinforced by posting of the UCLA EH&S 1-2-3 posters.

All UCLA research personnel have been trained to report all biohazardous incidents, injuries and near-misses, including NHP bites/scratches, to the UCLA Biosafety Office. To facilitate prompt reporting, Biosafety also supports a 24/7 reporting hotline. This requirement and procedure is reinforced by posting of the Biosafety A-B-C posters.

Similar postings advise those with personal health concerns or questions or who suspect potential occupational illness to contact the Occupational Health Facility for further evaluation, surveillance or special accommodations. The OHF staff regularly contact the Biosafety Officer to discuss any injuries involving biological materials and animals to ensure any potential hazards documented on IBC protocols can be addressed. The OHF tracks workman’s comp claims related to exposures and reports on them and can do ad hoc reports. The OHF also keeps logs of exposures to blood born pathogens and infectious agents.

The Office of Insurance and Risk Management (IRM) compiles a list of UCLA Workers’ Compensation claims made on a weekly basis and shares this information with the EH&S Injury/Illness Prevention Program (IIPP) Manager for further investigation. This is distributed among the EH&S safety division managers for identification and review of those involving hazardous materials (e.g., biohazards, recombinant DNA, chemical hazards) for root cause analysis and corrective action planning with the laboratory/research staff.

Any failure of engineering controls (e.g. HVAC failure) in the hazard containment areas, injury, illness, near-miss or non-compliance involving biological agents which may result in potential exposure risks (including NHP bites/scratches), along with the root cause analysis and corrective action plans is reviewed by the Institutional Biosafety Committee (IBC) at their twice monthly meetings. These are compiled into a table to enable further trend analyses and development and implementation of institutional-wide policies/practices based on hazards as identified. These research-related biohazardous material investigations are reported back to the IIPP manager for inclusion in IRM’s institutional injury tracking system.

DLAM has a safety officer and safety committee that reviews injuries and other safety-related incidents involving DLAM staff on a quarterly basis.

ii. Standard Working Conditions and Baseline PrecautionsThe following section pertains to the Occupational Health and Safety Program for all personnel associated with the animal care and use program. Specific

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information regarding the use of hazardous agents is included in subsection iii below.

1) Medical Evaluation and Preventive Medicine for Personnel [Guide, pp. 22-23] Note: Include blank forms used for individual health assessment as Appendix 6.

a) Describe who (e.g., personnel assigned to job/task categories in I.A.2.b.i.2) above) receives personal medical evaluation as a component of individual risk assessment. Describe who are not included and/or exempted from personal medical evaluation. Note: Do not include the names of personnel.

The occupational health and safety program is designed to include all personnel who handle animals, animal or human tissues, and hazardous agents in an animal research setting and/or maintain the animal facility. The degree of involvement in the program is based on specific hazard identification and risk assessment. In accordance with UCLA Policy 990, Use of Laboratory Animal Subjects in Research, all personnel involved in the care and use of research animals or their tissues must be enrolled in the program and are required to submit a Medical History Questionnaire (MHQ) annually for review by the Occupational Health Facility (OHF).

The vast majority of the above personnel participate in the occupational health and safety program via completion of the online questionnaire. In addition to the MHQ, DLAM personnel undergo an annual medical evaluation, annual testing and appropriate vaccination as a condition of employment and depending on work assignments, as follows: Tdap vacc. once and Td every 10 years (all) Tb questionnaire and annual testing via tuberculin skin test or

quantiferon blood test with follow-up (e.g x-ray) as required (all) Hep B vacc. (NHP and some cage wash workers; some ABSL2

workers) MMR vacc. (NHP and some cage wash workers) Influenza vacc. (NHP, swine and avian workers and some cage wash

workers) Rabies vacc (for bat areas; titer every 2 years) Other surveillance (e.g. vacc. relevant to a specific ARC protocol) as

directed by OHF

Research personnel working with biohazards may have specific vaccination or medical surveillance measures as conditions of IBC approval based on the agents they are working with.

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UCLA housekeeping staff are not permitted access to the DLAM animal facilities. Instead, DLAM performs all housekeeping services within the DLAM vivaria.

Any visiting personnel (e.g. Facilities maintenance workers) entering the animal facility are, at a minimum, briefed on appropriate precautions (either through the online DLAM General Awareness Training or in person by DLAM management staff), provided appropriate PPE, and are only permitted access to a specific area for a limited amount of time. A member of the animal care staff escorts visitors through the facility, and in most cases, and especially if there is extensive or prolonged maintenance work to be completed, animals are typically relocated prior to any work being initiated. Only in rare instances, i.e. where animals cannot be relocated or in an emergency when a DLAM escort is not available and a high risk area must be entered (e.g. NHP or hazardous containment area), more extensive training and medical clearance of visitors is required. There is a small group of Facilities emergency responders with full training (B virus, respirator fit testing, PAPR use, etc.) and medical clearance (including Tb testing, measles, rabies, influenza vaccination, etc.) available to work in high risk areas in the animal facilities.

Funds to cover lab animal Occ. Health medical evaluations, vaccinations, etc. by OHF for Facilities workers (and DLAM staff) are provided by UC Office of the President.

b) Describe provisions for allowing an individual to decline participation in all or parts of the medical evaluation and preventive medicine programs (if applicable). Provide an estimate (percentage) of personnel associated with the animal care and use program that have declined participation in the medical evaluation program.

In lieu of submitting the MHQ form, visitors (e.g. visiting researchers) may complete the MHQ Waiver Form (http://ora.research.ucla.edu/RSAWA/ARC/Documents/UCLA_MHQ_waiver_form.pdf ) provided they: 1) are not UCLA faculty, staff or students and 2) will only have transient contact with animals or animal or human tissue for a period of time not to exceed 3 days. All others must complete the MHQ.

All personnel who are at risk of exposure to human-source materials legally must be offered the Hepatitis B vaccine. If they choose to decline this vaccine, they must complete a declination form.

For research staff, those vaccinations/surveillance measures that are solely or primarily for the purposes of human health and safety (e.g., HBV or Tdap

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vaccinations) and do not present any human public health pandemic risk as determined by the IBC risk assessment, may decline participation in the medical evaluation and preventative medicine programs with hazard communication documentation and a signed waiver.

With the above exceptions, the OHF Director is not aware of any research staff or DLAM staff who have declined participation in the medical evaluation program for animal users at the time of the writing of this Program Description.

c) Describe provisions for assuring confidentiality of medical information.

Confidential medical information is handled by medical professionals who are HIPAA trained. The OHF records are maintained under the UCLA Health Systems medical records and are separate from any HR or personnel files that supervisors may access.

If special accommodations or temporary restrictions are recommended by the OHF based on personal health issues, only the conditions/restrictions are communicated, not the personal health information (PHI).

All investigations and reports which may undergo safety committee review are scrubbed from names of any individuals for de-identification purposes.

d) Describe safety considerations for individuals with incidental exposure to animal care and use (e.g., contractors, personnel working in open laboratories).

Contractors and other visitors receive escorted access through DLAM animal facilities and are provided General Awareness Training and/or medical clearance as described above in section ii.1.a).

On an annual basis, the ARC administrative office distributes an EH&S Fact Sheet about laboratory animal allergens and occupational asthma with the intention of the announcement and attached fact sheet being made available to all personnel in labs, not just those that work with animals. This and other Facts Sheets encourage individuals (e.g. in open laboratories) to self-report any health concerns to the Occupational Health Facility. The ARC encourages all labs to print and post the flyer in a conspicuous place.

In January 2017, the AVC for Laboratory Safety distributed a memo to the research community regarding personal health conditions impacting safety in laboratories. The memo contained a link to a fact sheet that provides important information about making accurate biosafety risk assessments that may change with changing health status. Personnel with questions

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about whether their health status represents a risk in working with organisms in their laboratory situation are encouraged to contact OHF to request a confidential appointment.

e) Describe general features of the medical evaluation and preventive medicine programs, within the context of work duties, including: • pre-employment/pre-assignment health evaluation,• medical evaluations (including periodicity),• diagnostic tests (e.g., for tuberculosis),• precautions for working with potentially hazardous species (e.g.,

nonhuman primates, sheep, venomous species)• immunization programs, and• procedures for communicating health related issues.

The risk assessment and need for health care services is a collaborative professional judgment of all interested parties including: the AV, who is knowledgeable about zoonotic risks; a medical care provider from OHF; a specialist from EH&S who is knowledgeable about occupational hazards; the IBC for evaluation of zoonotic risks and/or involving biohazardous research materials; and/or the principal investigators who can assess the health risks associated with their planned experimental protocols.

At a minimum, in most cases, personnel submit an annual MHQ online for review by the medical staff at the OHF. The ARC database is updated whenever clearance of individuals listed on animal use protocols is granted or withheld. The ARC staff provides individuals with 90-day notifications of impending MHQ expiration.

Any health restrictions are evaluated by the Occupational Health Facility (OHF) professionals and individuals affected are notified.

DLAM staff are evaluated upon hiring and annually as described in section b.ii.1.a (~p. 28).

There may be special vaccinations/surveillance for anyone working with some biological agents used in research (e.g., vaccinia, strep pneumo) and some species or agents (e.g. rabies vaccine for those working with bats, TB testing for those working with NHPs or TB material, etc.).

Personnel are advised either during EH&S training or while completing the MHQ that, if they are pregnant, may be pregnant, or are planning to become pregnant; are ill; or have a medical change which may result in impaired immune-competence, they should consult a health care professional/physician regarding such conditions and how they might pertain to their working with laboratory animals or in areas where

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laboratory animals are used. If warranted, any work restrictions and/or accommodations are coordinated among the individual, his/her health care professional, the occupational health services and human resources. This includes inability to use/wear PPE, conditions which may provide portals for pathogen entry, etc.

UCLA is currently piloting a program developed at the UC-system-wide level, called the Occupational Health Surveillance System (OHSS). The OHSS involves a multi-step assessment of personalized risks: (1) The supervisor creates a Risk Assessment (RA) for the Participant. (2) The participant reviews the RA and accepts or rejects if changes are needed. (3) After accepting the RA, participant fills out the confidential Health Questionnaire (HQ) and submits for review by health professional. Personnel are advised to have their vaccination history available as vaccine dates are requested on the HQ. (4) The Health Professional reviews the participant’s RA and HQ and sends a medical assessment for the participant to review. (5) The participant logs into OHSS and reviews / acknowledges the medical assessment. If there are questions from the health professional on either the HQ or RA, or services are needed, a response from the participant will be needed to complete the process. Emails are sent after each step. This process may eventually replace the MHQ for some or all personnel associated with the animal program or facilities.

f) Describe any other entities that provide medical services (e.g., emergency care, after-hours care, special medical evaluation, contracted services). Include a brief description of their credentials and/or qualifications, and how these entities remain knowledgeable about animal- or institution-related hazards and risks.

Emergency medical treatment may be provided by the Ronald Reagan UCLA Medical Center emergency department, if incidents occur outside of OHF business hours. Licensed emergency department (ED) professionals are provided training with their supervisor on the USAMRIID manual. ED staff/RRUCLA Emergency planning are included in annual High Containment Incident Response training from high containment laboratory, which includes the response for TB incidents. ED staff are instructed to refer occupational health exposures to OHF for follow-up. Currently, Facilities and most EH&S personnel are on-boarded through Brentview Medical—a contracted medical provider (once OHF gets its new clinic and staffing, the hope is that Brentview will be phased out). In some circumstances involving biohazardous materials that are not normally seen in the community (e.g., recombinant viruses and/or NHPs), the IBC requires the lab to have post-exposure plan documents and lab staff are advised to bring these with them to the health care provider to ensure proper communication and procedures.

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2) Personnel Training Regarding Occupational Health and Safety [Guide, p. 20]

Describe general educational program(s) to inform personnel about: allergies, zoonoses, personal hygiene, physical injuries in animal facilities (e.g., noisy areas, large

quantities of chemicals such as disinfectants, ergonomics) or species used (e.g., nonhuman primates, agricultural animals),

other considerations regarding occupational health and safety.

Include in the description a summary of the topics covered, including: Entities responsible for providing the training Frequency of training or refresher training

Note: Do not include special or agent-specific training for personnel exposed to experiment-related hazardous agents; this will be provided in Section iii.3 below.

Information on zoonosis, allergies, and other general occupational risks associated with the animal facility, is provided to the investigators and their staff starting with the CITI module “Occupational Health and Safety (ID:13352)” which is part of the general required CITI training course. Additional required CITI species-specific courses provide additional information according to species. In addition, during DLAM-taught species-specific classes, personnel are instructed on physical risk (scratch, bite), zoonosis and allergens, and how to respond to incidents at UCLA. Research staff take the general CITI refresher course training every 3 years.

For DLAM employees, there are periodic all staff hands on training, or lectures associated with safety. These are taught by EH&S or DLAM Supervisor or veterinary staff. Topics discussed include risks when working with laboratory animals, allergies, hazardous spills, needle sticks, and emergency exit from walk-in cage washers and autoclaves. DLAM employees working with hazardous chemicals receive training on the chemical’s MSDS and associated EH&S SOPs. MSDS and/or SOPs are generally kept in binders in those areas where the chemicals are used, mainly cage wash.

General awareness training, provided online by DLAM, is required for any non-researcher staff including maintenance employees prior to getting access to the vivarium. This training includes components on occupational health including zoonosis and allergies.

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For employees working in hazardous containment areas, but not directly with the agents, agent summary sheets (provided by EH&S) are posted at the door in each room addressing specific PPE and response to exposures.

ARC, DLAM and EH&S provide more specific training/education on zoonotic risks of some species. These include: The online B virus training through Worksafe. Hazard communication related to Mycobacterium marinum

(https://ucla.box.com/v/MmarinumRisks) Lab Animal allergies & Occupational Asthma fact sheet

(https://www.ehs.ucla.edu/doc/lab-animal-allergies-occupational-asthma/at_download/file)

Personal Health Risks in Laboratories fact sheet (distributed; not yet posted on EH&S website).

3) Personal Hygiene [Guide, p. 20; Ag Guide pp. 4-5]

a) List routine personal protective equipment and work clothing provided and/or required for animal care personnel, research and technical staff, farm employees, etc.

DLAM technical staff are provided uniforms, scrubs (short-sleeve scrub tops and pants) and/or lab coats to wear during their work shift. UCLA Shoes For Crews Program provides all technician staff dedicated slip-resistant work shoes; assigned shoes are eligible to be replaced every 6 months. Lockers are provided for storing street clothes and personal belongings. Shower facilities are available, along with laundered towels; technical staff are encouraged to shower at the end of their work shift. There are enough uniform/scrubs/coats assigned to change into freshly laundered uniforms/scrubs/coats on a daily basis.

In DLAM vivaria, standard disposable PPE is typically provided in the facility by DLAM for both DLAM staff and researchers. Non-disposable or PPE related to operationally-specific procedures (e.g., PAPRs) are the responsibility of the researchers to bring to the DLAM vivarium.

For most small animal facilities, the minimum PPE required to enter is a disposable long-sleeved gown and gloves when handling animals. Certain work areas require additional PPE, such as hair covers and masks when working with immunodeficient rodents; or hair covers, masks, shoe covers, and a second pair of gloves when working with biohazards in rodent areas. Signs are prominently posted (facility/suite entrances and/or on animal room doors) to indicate the PPE requirements.

Hazard- or operational-risk based PPE is assessed during IBC, RSC, CHO or Laser Safety review processes.

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b) Describe arrangements for laundering work clothing.

Laundry services are contracted and provided by an industrial laundering service vendor (Mission Linen Supply Inc.). Soiled uniforms or lab coats are collected and clean uniforms are delivered weekly.

c) Describe provisions and expected practices for washing hands, showering, and changing clothes, including instances where work clothes may be worn outside the animal facility.

Showers and change facilities are located in the major DLAM animal facilities. Sinks are located in some animal holding rooms, all procedure rooms, some corridors and all restrooms for washing hands. Clean DLAM scrub uniforms may be worn into staff lounge areas, and limited on and off-campus areas. Soiled scrubs must be changed and left in the hampers before entering public areas or leaving for home. Again, DLAM staff are encouraged to shower before they leave for the day in order to minimize transfer of allergens to their households.

d) Describe policies regarding eating, drinking, and smoking in animal facilities.

Eating and drinking within animal facilities is only permitted in designated staff lounge areas. Smoking is not permitted within any University structure, including animal facilities and laboratories.

4) Standard Personnel Protection [Guide, pp. 21-22]

a) Describe facility design features, equipment and procedures employed to reduce potential for physical injury inherent to animal facilities (e.g., noisy areas, large quantities of chemicals such as disinfectants, ergonomics) or species used (e.g., nonhuman primates, agricultural animals).

To reduce the potential for physical injury inherent to animal facilities and species used, DLAM works closely with EH&S to identify high risk areas or activities and employ a number of appropriate engineering controls. To help control airborne hazards DLAM facilities must maintain a minimum air changes per hour, inward directional air flow, individually ventilated caging, and laminar flow work stations or biosafety cabinets. To assist in safely working with animals and equipment, DLAM facilities have minimum lighting requirements as appropriate for the area. To help prevent slips and falls DLAM areas have slip-resistant finishes on floors and DLAM staff are provided slip-resistant shoes. To combat fatigue and prevent

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muscle and ergonomic injuries DLAM employs anti-fatigue mats, a power tug to move large equipment, water bottle stoppers to replace twist-style caps, modified pig grates (to minimize heavy lifting during husbandry), modified manual bedding filler used to fill rodent cages, ergo-carts for transporting cages, racks for water bottles, and feed barrels used within rodent vivarium (specially constructed to minimize bending). There are many other examples of controls, used for miscellaneous risks, such as emergency cage wash exit mechanisms in all our washers, modified NHP caging to allow for safe transferring of NHPs from housing enclosure to play cage, and sharps containers in the procedure rooms and many of the animal holding rooms.

In addition to engineering controls used to reduce the potential for injury, DLAM works with EH&S, the ARC and IBC to develop administrative controls (SOPs and training), as well as requirements for PPE appropriate for the work environment. As part of the department Injury Illness and Prevention Program (IIPP), instruction in safe ergonomic procedures, injury prevention and reporting is provided during initial orientation of new DLAM personnel and throughout the year as part of quarterly IIPP meetings. Also, staff members are provided education at least annually on: Emergency cage wash exit mechanisms Hearing protection and use of disposable ear plugs or muffs in cage

wash, swine and dog areas Sharps containers and responding to needle stick, animal bites or scratches Spill cleanup procedures Zoonoses Bloodborne Pathogen awareness and emergency response Disaster Plan

trainingAt least annually, EH&S provides ergonomics training on proper lifting, pulling, pushing techniques during one of the “All DLAM Staff” monthly meetings. To help avoid bites and scratches all personnel who work with animals must provide evidence of experience and training to safely handle animals and perform their duties, or such training is provided by DLAM. Finally, all personnel entering or working in the animal facility are required to wear appropriate PPE for the area which may include disposable gowns and gloves, thick gloves for working with hot items, aprons and face shields to prevent chemical injuries, Tyvek or neoprene sleeves, face shields and goggles when working with NHPs, and hearing protection when required, etc. PPE requirements are described in DLAM SOPs, posted in the animal facility, and presented in researcher training seminars.

DLAM facilities are inspected twice yearly by either the DLAM Safety Officer or by Lab Safety (targeted inspections) to evaluate high risk areas and activities such as storage and transfer of chemicals/disinfectants,

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electrical safety, etc.

EH&S office has conducted risk assessments including lab animal allergens, anesthetic exposure and noise levels. Reports are available for review by the site visit team.

b) Describe likely sources of allergens and facility design features, equipment, and procedures employed to reduce the potential for developing Laboratory Animal Allergies (LAA).

The potential for developing LAA, which would be predominantly to airborne or contact-spread animal dander and urine proteins, especially rodents, is well-recognized and prevented and controlled by engineering and administrative controls as well as PPE. To minimize the amount of allergen material in the environment, we have/use minimum air changes per hour, directional air flow in the animal rooms, micro-isolator and/or individually ventilated caging, and biosafety cabinets or laminar flow work stations. All personnel who work with animals, or work with animal materials or caging, are experienced and trained to safely handle animals and perform their duties. All personnel entering or working in the animal facility are required to wear appropriate PPE for the area which may include disposable gowns and gloves (latex alternates are available for those with latex allergies), fit-tested respiratory protection and hair covers as appropriate (e.g. for anyone with allergies and changing rodent cages outside of a change station and for DLAM staff where soiled cages are dumped). PPE requirements are described in DLAM SOPs, posted in the animal facility, and presented in researcher training seminars.

c) Describe likely sources of zoonoses and facility design features, equipment, and procedures employed to reduce potential exposure to zoonoses.

Potential zoonoses of concern are B Virus and Tuberculosis, Measles, Methicillin-resistant Staph. aureus, Flu, SIV, pox virus, filoviruses, Salmonella, Shigella and Chagas Disease in non-human primates; Rabies, Ringworm, Roundworms and Rickettsial diseases in dogs; E. rhusiopathiae, Pseudorabies, brucellosis, Flu, Salmonella, E. coli and Leptospirosis in pigs; Ringworm and Tularemia in rabbits, Chlamydia psittaci, Histoplasma capsulatum, and Cryotococcus neoformans in birds, M marinum in aquatics, and Mycobacterium avium and Rabies in bats. Potential zoonosis associated with field studies would be identified and risks addressed via consultation between the OHF Director and researchers involved in the field studies. In general, zoonoses are prevented by appropriate practices (SOPs), training and PPE. All animal vendors are screened and approved, based in part on health history and diagnostic

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surveys, prior to first shipment and at regular intervals thereafter. Quarantine upon arrival is required for some species such as NHPs and rodents from non-approved vendors. Diagnostic testing is performed for many potentially zoonotic agents in quarantine (e.g. Tb for NHPs) and regularly thereafter in some colony animals, depending on species (e.g. rodent sentinels, Rabies testing in found-dead bats). Complete details of these practices and more can be found in our preventative medicine SOPs: Animal Biosecurity, Quarantine and Stabilization, Separation by Health Status and Species, Surveillance, Diagnosis, Treatment and Control of Disease.

Facilities are designed with safety in mind (secured access; HVAC capable of 10-15 ACH, ability to hold negative pressure; trench drains in large animal rooms to assist with sanitation, etc.). Zoonoses training is provided in the species-specific online training modules required by the ARC. Additional special training, e.g. Blood borne Pathogens and B Virus Exposure training for NHPs is required and provided as appropriate. PPE requirements in the animal facilities range from a minimum of disposable gown and gloves where zoonoses risks are small (e.g. rodents) to ABSL2 requirements where risk is greater or consequences of infection are more serious (e.g. NHP and bats). Rabies prophylaxis is required of anyone working with bats. Finally, all discovered potentially zoonotic agents are reported to EH&S which typically results in additional training of DLAM and research staff, signage and PPE until the threat has been resolved.

d) Describe the procedures for the maintenance of protective equipment and how its function is periodically assessed.

Equipment maintenance is completed at scheduled intervals. For example: Respirator fit testing and certification is completed annually Slip resistant shoes are replaced every 6 months Moveable equipment (tugs, racks and carts) is assessed routinely and

wheels and moving parts are greased/lubricated or replaced as needed Laminar flow hoods, chemical fume hoods, dumping stations,

ventilated rack system blowers (in hazardous containment areas) and biosafety cabinets are all certified at scheduled intervals (1-3 years or when moved or in preparation for GLP studies)

e) Respiratory Protection

i) Describe situations where respiratory protective equipment is available or required, such as cage washing facilities, feedmills, etc.

A fit-tested N95 respirator is provided and required of personnel dumping soiled rodent cages in all of our facilities and for changing

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cages in Franz Hall (where no laminar flow change station is provided). Also, respiratory protection is required for certain procedures involving NHPs, such as surgery using drills or spray washing cages and equipment, where potentially hazardous material may become aerosolized; also TB use and bat areas.

ii) Describe programs of medical clearance, fit-testing, and training in the proper use and maintenance of respirators.

EH&S Industrial Hygiene Office coordinates the UCLA Respiratory Protection Program (RPP). This involves: Completion of a Respiratory Hazard Assessment form

(https://www.ehs.ucla.edu/doc/RespiratoryHazardAssessmentForm.pdf/view) is required to enroll in the respiratory protection program. In addition, the IBC and/or CHO review hazards and operations as part of their review to make recommendations for respiratory protection.

In-person training on the use, care, maintenance and storage of respirators. Three regular in-person classes are offered for N95 masks, half-face respirators and full-face respirators, as appropriate. PAPR training is typically provided through the High Containment Director.

Medical clearance is coordinated through the Occupational Health Facility as part of these in-person training classes. Personnel complete the OSHA respirator health questionnaire intended to identify potential personal health concerns which may preclude safe respirator use. These are reviewed with an Occupational health care provider from OHF to obtain clearance.

Qualitative fit-testing is performed for each staff member for N95 masks and half-face respirators. Quantitative fit testing is performed for full-face respirators.

Annual medical clearance and fit testing (or when facial structure changes may have occurred) is required for those enrolled in the RPP.

EH&S offers the following in-person training: Half-Face and other Cartridge Respirator Training and Fit Testing N95 Respirator Training and Fit Testing

iii) Describe how such respiratory protective equipment is selected and its function periodically assessed.

Selection of respiratory protection is based on the hazards in the facility. The hazards and risks are assessed by EH&S staff- either in conjunction with an ARC or IBC review process (in the case of chemical or

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biohazardous materials use), or based on surveillance of areas and operations (e.g., laboratory animal allergen testing by industrial hygiene).

Once a need for respiratory control has been identified, all personnel must complete a Respiratory Hazard Assessment Form for review by the EH&S Industrial Hygiene staff. The options of models for facial differences and preferences of the wearer are also taken into account during selection.

All respirators are required to be fit-tested at least annually, typically using a qualitative fit test by the Industrial Hygiene staff. Personnel are also taught and advised to spot-test their respirators during donning procedures in the annual training courses provided by the Industrial hygienist.

f) Heavy Equipment and Motorized Vehicles

i) Provide a general list of the types of cage-processing equipment used, such as rack/cage washers, tunnel washers, robotics, and bulk autoclaves. Describe training programs, informational signage, and other program policies designed to ensure personnel safety when working with such equipment.Note: Details of specific equipment installed in animal facility(ies) are to be provided in Appendix 15 (Facilities and Equipment for Sanitizing Materials).

There are a total of 10 Rack washers, 6 tunnel washers and 14 sterilizers in 11 animal facility areas (including Radiation Oncology, which we include in this program description as a Study Area). All cage washing machines are equipped with emergency shutoff/exit mechanism as well as heat/moisture resistant exit signs; Emergency off button and lockout key are safety features for bulk sterilizers.

Training for cage wash personnel is covered by a Standard Operating Procedure. The Cage Wash Training SOP includes directions for training personnel on safety procedures, including: Correct methods to lift, push and pull heavy items Correct use of PPE Proper loading/unloading and handling hot items from autoclaves Locations of emergency exits, eye wash stations, showers, fire

extinguishers, and first aid kits Emergency shut-off procedures for equipment such as tunnel

washers Emergency shut-off and exit procedures if trapped inside a rack

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washer

ii) List other heavy equipment such as scrapers, tractors, and farm machinery (manufacturer name, model numbers, etc. are not necessary). Describe training programs, informational signage, and other program policies designed to ensure personnel safety when working with such equipment.Note: If preferred, this information may be provided in a Table or additional Appendix.

None

iii) If motorized vehicles are used for animal transport, describe how the driver is protected from exposure to hazards such as allergens or zoonoses and decontamination methods employed. Also describe instances where vehicles may be shared between animal and passenger transport.

DLAM vivarium’s fleet has 4 vehicles: 2 pickup trucks with open bed, these are primarily used to transport equipment and supplies - 1 box truck with A/C dedicated for animal transport and – 1 transport van which is primarily dedicated for transporting personnel. All animals are transported in the box truck. While large animals may be transported in open crates, the cargo compartment of the truck is completely separated from the driver’s compartment. Rodents are transported in shipping crates or inside static micro isolator cage (water bottles removed) placed in dark color paper or plastic bag. A/C is kept running while the animals are in the vehicle. The area where animals’ crates/cages are kept during transport will have debris swept, sprayed with disinfectant and wiped off (*refer to Appendix 14). DLAM personnel who transport animals and disinfect the box truck wear scrubs and dedicated shoes. When disinfecting the truck, they also wear goggles or face shield w/ splash protection. They change scrubs daily, and are encouraged to shower before changing into their street clothes at the end of the work day. DLAM has an SOP that addresses transport in vehicles (Rodent Transport) and the ARC has a policy that covers this topic (http://ora.research.ucla.edu/RSAWA/ARC/Pages/ARC-policies/animal-transport.aspx)

g) Describe safety procedures for using medical gases and volatile anesthetics, including how waste anesthetic gases are scavenged.

If volatile anesthetic agents are administered via a precision vaporizer, waste anesthetic gases are scavenged using the following hierarchy of safety methods, with active capture/scavenging preferred over passive

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capture. The Best method is to work in a certified chemical fume hood or

certified hard-ducted (Class IIB2) biosafety cabinet. The next best is Active scavenging devices (ducted): WAG collection

devices (i.e., exhausted induction chamber and/or surgery nose cone, snorkel trunk) which is ducted to the building’s exhaust system. We do NOT use the lab vacuum as a means of active scavenging, unless approved by EH&S (EH&S and FM are evaluating the feasibility of using the building vacuum systems. Until then, they are not used).

Any building exhaust system (i.e., fume hood, snorkel, BSC) used to prevent harmful exposure is tested at least annually as required by Cal/OSHA. When the WAG collection devices noted above cannot be ducted to the building exhaust system, we use a manufacturer recommended air cleaning extraction system with an activated charcoal adsorption unit to actively scavenge WAG. We certify system according to manufacturer’s recommendation. Passive charcoal canister capture relies on positive pressure from the anesthesia machine and the anesthetized animal’s exhalation to push WAGs into gas adsorption units (i.e., canisters). Any leaks in passive scavenging systems, due to, for example, an inadequate seal on the induction chamber cover or particularly with tubing and nose cones can cause WAG to leak into the work area.

If volatile anesthetic agents are used without a precision vaporizer, procedures must be performed within in a chemical fume hood, an externally-ventilated biosafety cabinet (i.e. Class II B2), or in a well-ventilated area, with at least 6 room air changes per hour (ACH; this last method is highly discouraged and seldom allowed). We ensure air from this area is 100% exhausted and not recirculated to any other areas. A risk assessment (coordinated between EH&S and ARC or DLAM) is required for practices outside of the parameters listed above.

iii. Animal Experimentation Involving Hazards [Guide, pp. 20-21]

1) List, according to each of the categories noted below, hazardous or potentially hazardous agents currently approved to be used in animals that are or will be maintained for more than a few hours following exposure. If the hazardous agent cannot be listed by name for security/proprietary reasons, identify it by the general category of agent and level of hazard. Note: If preferred, this information may be provided in a Table or additional Appendix.

a) Biological agents, noting hazard level (CDC Biohazard Level, Directive 93/88 EEC, CDC or USDA/DHHS Select Agent, etc.). Examples may include bacteria, viruses, viral vectors, parasites, human-origin tissues,

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etc.

See Appendix 19 for a list of biological agents currently listed on an active ARC protocol.

b) Chemical agents, noting general category of hazard (toxicant, toxin, irritant, carcinogen, etc.). Examples may include streptozotocin, BrdU, anti-neoplastic drugs, formalin, etc.

See Appendix 20 for a list of chemical agents currently listed on an active ARC protocol.

c) Physical agents (radiation, UV light, magnetic fields, lasers, noise, etc.).

Radiation Magnetic fields (MRI) Electrical fields (ablation equipment) Ultrasound Lasers UV light Noise

2) Experiment-Related Hazard Use [Guide, pp. 18-19; See also Chapters 2 and 3 in Occupational Health and Safety in the Care and Use of Research Animals, NRC 1997]. Note: Written policies and standard operating procedures (SOPs) governing experimentation with hazardous biological, chemical, and physical agents should be available during the site visit.

a) Describe the process used to identify and evaluate experimental hazards. Describe or identify the institutional entity(ies) responsible for ensuring appropriate safety review prior to study initiation.

The institutional entities responsible for ensuring appropriate safety review prior to study initiation include the Institutional Biosafety Committee, EH&S Chemical Safety Division, EH&S Radiation Safety Division, and/or Occupational Health Facility.

Potential hazards are identified by a combination of methods including: (1) Review of ARC, IBC, and radiation use applications; (2) laboratory and vivarium visits by EH&S, ARC and DLAM personnel; (3) department safety coordinator meetings; (4) DLAM has a safety officer, whose duties include evaluating and mitigating hazards and risks involved with animal use; (5) the DLAM safety officer attends monthly IBC meetings and coordinates communication between EH&S, IBC and DLAM and researchers to ensure

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identification and mitigation of hazards.

ARC protocol review includes review of safety issues, and consultation between the researchers and EH&S subject matter experts to ensure that safe procedures are followed. As a result of ARC and IBC protocol reviews, agent summary sheets are generated for each hazardous agent used in animals. These sheets are posted at the doors of rooms in which hazardous agents are used in animals, so that all personnel have access to the information before they enter the room.

Finally, researchers are required to enroll in the Occupational Health Program for laboratory animal users, by completing the online Medical History Questionnaire (MHQ), before being added to an animal use protocol. In accordance with University Policy, completion of this form, which includes questions about experimental hazards, is mandatory for all personnel having contact with research animals or animal tissues and/or all personnel who have a security key card or key to enter the DLAM vivarium. UCLA is exploring implementation of a UC system-wide program, the Occupational Health Surveillance System, to replace and expand the evaluations performed by the MHQ.

b) Describe how risks of these hazards are assessed and how procedures are developed to manage the risks. Identify the institutional entity(ies) responsible for reviewing and implementing appropriate safety or containment procedures.

The UCLA Biosafety or Chemical Hygiene Officer performs Risk Assessments and the Institutional Biosafety Committee (IBC) or EH&S Chemical Safety Division reviews, assesses potential dangers, and approves or denies the use of hazardous agents. A review of procedures involving hazardous agents also occurs during protocol review by the ARC. EH&S and DLAM supervisory staff are responsible for training of personnel and oversight of potentially hazardous biologic, physical, and chemical agents. The EH&S Radiation Safety Division is responsible for training and oversight of laboratories using radiation or radioactive isotopes as part of their experimental protocol. The aforementioned EH&S offices conduct laboratory inspections to assure compliance with applicable laws and regulations and work closely with vivarium management to ensure proper containment of hazards and adequate labeling of rooms and areas that may pose a potential risk. These offices make it clear to researchers that the Principal Investigator is ultimately responsible for compliance by members of their laboratories.

Such hazards are reassessed during ARC, IBC, and EH&S reviews, as well as during the annual Medical History Questionnaire (MHQ) review, performed by the Occupational Health Facility (OHF).

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c) Describe the handling, storage, method and frequency of disposal, and final disposal location for hazardous wastes, including infectious, toxic, radioactive carcasses, bedding, cages, medical sharps, and glass.

Needles/sharps containers are placed in each procedure room and in holding rooms wherever needed. Sharps containers are closed when ¾ full and disposed as medical, trace-chemotherapeutic or radioactive waste, as appropriate.

Trash/refuse, disposable caging/bedding and carcasses that may have been exposed to and/or contaminated with human materials or other hazardous animal cells/tissues/fluids, recombinant materials or from animals treated with chemotherapy agents are treated as medical wastes. Medical wastes are placed in appropriate colored medical waste bags, sealed, and placed in a medical waste container with proper labels as per state regulations. Medical waste is then transported to a designated accumulation site for transport and treatment by a permitted medical waste vendor.

Medical waste carcasses deemed hazardous (containing formalin, or animals exposed to BSL2 agents, for example) are placed in dedicated refrigerators or freezers within hazardous containment areas. These are then transported by trained DLAM staff to the biohazard carcass freezer located in the hallway at 1V150, for collection and incineration by a commercial contractor.

All radioactive waste is under the jurisdiction of the UCLA Radiation Safety Officer (RSO) who handles/picks up waste.

d) Describe aspects of the medical evaluation and preventive health program specifically for personnel potentially exposed to hazardous agents.

Researchers are required to enroll in the Occupational Health Program for laboratory animal users, by completing the online Medical History Questionnaire (MHQ), before being added to an ARC protocol. Experimental hazards are covered by the MHQ and preventative measures, such as vaccinations, may be identified at the time of MHQ review.

Protocols involving hazardous agents are reviewed by subject matter experts during Committee review and preventative measures may be discussed at that time. For biohazardous materials identified during the IBC-review process the IBC may add stipulations for preventative medical measures or surveillance as a condition of the IBC approval. In addition, the IBC will ask that PIs identify special precautions or risks for those with risk of infection or for whom consequences may be increased on the IBC protocol, as well as

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develop post-exposure plans as part of their Biosafety Manuals.

If the research is to take place within the DLAM hazardous containment areas, the two DLAM staff members who serve on the IBC are asked to review these measures to ensure provisions can be made to protect DLAM staff members if they are expected to care for these animals (DLAM staff generally do not care for animals exposed to carcinogens, toxins and chemical hazards). Otherwise, the IBC stipulates that PI staff must care for these animals, and have SOPs related to this care.

Bite/Exposure kits are placed in all macaque NHP housing and procedural locations, including all locations where macaque NHP tissues are used. Potential exposures are handled in accordance with the current guidelines from the NIH B Virus Resource Laboratory.

Finally applicable Safety Data Sheets (SDS) are posted anywhere infectious agents, human origin tissues, or hazardous chemicals/toxins/poisons are being utilized. Precautions, special handling and PPE requirements are reviewed and communicated to personnel working within these locations.

3) Hazardous Agent Training for Personnel [Guide, p. 20] Describe special qualifications and training of staff involved with the use of hazardous agents in animals.

Personnel working with hazardous agents are required to complete the following training through EH&S, as appropriate to their work:

Institutional Biosafety Committee (IBC) Compliance training Medical Waste Management Bloodborne Pathogens Biological Safety Cabinet Biosafety A, B, Cs – Biosafety Level 2 Biosafety Level 2 with Biosafety Level 3 Practices (BSL2+) Biosafety Level 3 Shipping Biological Materials B-Virus Exposure Online training Laboratory Safety Fundamental Concepts Laboratory Safety for PIs and Lab Supervisors Laser Safety training N95 Respirator Training and Fit Testing New Radiation Worker Qualification X-Ray Diffraction Safety Training

In addition to completing training, personnel must be approved for hazard work under the appropriate safety committee protocol corresponding to research

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described in the ARC protocol.

Before being added to an animal use protocol, all researchers are required to take the online Collaborative Institutional Training Initiative (CITI) basic animal welfare course, which discusses use of hazardous agents in animals, as well as hazards inherent in working with animals (allergies, bites etc.).

DLAM requires online training for research staff working in the hazard containment facilities. DLAM also trains containment facility staff which includes discussion of potential and specific hazards (including Safety Data Sheets), Right to Know (location and function of Safety Data Sheets), methods to protect against such hazards, and procedures to be followed in the event of a spill or an exposure.

4) Facilities, Equipment and Monitoring [Guide, pp. 19-20]

a) Describe locations, rooms, or facilities used to house animals exposed to hazardous agents. Identify each facility according to the hazard(s) and containment levels (if appropriate). Note: If preferred, information may be provided in a Table or additional Appendix.

Animals exposed to biohazardous agents and some chemical hazards are housed within a designated hazardous containment facility or area/room. Animals are not permitted to be removed from hazardous containment areas without approval from the Institutional Biosafety Committee or Chemical Safety Officer. Engineering controls, administrative controls, and PPE are required and available in all hazardous containment areas. Radioisotopes and chemical hazards used in animals require housing in separate, specific rooms and/or racks identified and properly labeled prior to onset of the experiment. All hazardous cages regardless of hazard type are identified with appropriate hazard stickers on the cage cards.

Locations in the vivarium that are approved for ABSL2/2+ work, and hazards examples, include:

Location HazardsCHS AR-173 (DLAM; ABSL-2/2+)

Human cells, Radioactive agents, Recombinant viral vectors (lenti-, adeno-, mouse retroviral), Murine Herpes Virus–68 (MHV-68), Cyclophosphamide, Doxorubine, Pactaxel Methotrexate, several other Chemo drugs

CHS 1V518 and 1V515 (DLAM; ABSL-2)

Strongyloides ratti, Nippostrongylus brasiliensis, Strongyloides stercoralis; Ancylostoma ceylanicium, Parastrongyloides

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trichosuriCHS 2V-111 (DLAM; ABSL-2)

Human cells; Recombinant, replication competent retroviral vectors; recombinant lentiviral vectors

CHS 2V-135 (DLAM; ABSL-2)

Human cells; cyclosporine in rabbits

CHS 4V- 4V514 (DLAM; ABSL-2)

Gnotobiotic work- human cells, human fecal material, Akkermansia muciniphilia

CHS 3V Biocontainment Facility (DLAM; ABSL-2/2+)

Human and other mammalian cells, Non-recombinant viruses and recombinant viral vectors (lenti-, adeno-, retro-, including HIV, SHIV), Recombinant murine Herpes Virus–68 (MHV-68), MCMV, HCMV, Influenza virus (A/WSN/33 or 34, PR8), Listeria Monocytogenes, LCMV, Bilophila wadsworthia, Streptococcus pneumoniae, Salmonella typhimurium, Modified (G-deleted) rabies virus, Mycobacterium bovis BGC vaccine strain, Mycobacterium bovis, Mycobacterium avium, Mycobacterium leprae, Mycobacterium microti, Mycobacterium smegmatis, Yersinia pestis (Pgm- attenuated strain), Mycobacterium tuberculosis, Peptostreptococccus micros, Yersinia enterocolitica, Klebsiella pneumoniae, Staphylococcus aureus (including MRSA strains), Staphylococcus epidermidis, Staphylococcus sanguinis, Streptococcus intermedius, Treponema denticola, Eschericia coli (enteroinvasive and enteropathogenic), Francisella tularensis LVS strain, Francisella novicida, Vibro vulnificus, Rhizopus oryzae, Propionibacterium acnes, Porphyromonas gingivalis, Fusobacterium nucleatum, Prevotella inermedia, Pseudomonas aeruginosa, Vescicular Stomatitis Virus (non-exotic) Indiana 1 strains, Bordetella pertussis, Bordetella bronchiseptica, Bordetella parapertussis, Bacteroides spp., Legionella pneumophila, Zika virus, Paramyxovirus Pneumonia Virus of Mice (PVM), Chlamydia muridarum, Chlamydia trachomatis, Clostridium difficile, Akkermansia muciniphilia, Haemophilus pneumoniae, Moraxella catarrhalis, Heligmosomoides polygyrus, Ancylostoma ceylanicum, Strongyloides papillosis, Picornavirus Human enterovirus-coxsackie virus B3, Picornavirus

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human enterovirus-Parechovirus (HpeV1), Saccharomyces boulardii, Blautia coccoides, Anaerostipes caccae, Vaccinia virus, Neospora canium, Acinomyces naeslundi, Anaerostipes caccae, Toxoplasma gondii, various Chemo drugs, Carcinogens, Nanoparticles, MPTP

CHS 6V-133 (PI-Iwamoto Maintained; ABSL-2)

Human cells, Recombinant viral vectors (lenti-, retro-, Adeno-), Biolophila wadsworthia, Lactobacillus johnsonii, Helicobacter hepaticus, Porphyromonas gingivalis.

CHS 8V342 and 8V324 (DLAM; ABSL-2)

This is the location for hazardous pigs. Chemicals (e.g., cyclosporine) and Human cells used in these locations

CNSI 2130 Suite- Crump Imaging Facility Housing (DLAM; ABSL-2/2+)

Human cells, Recombinant replication-defective viral vectors (lenti-, retro-, adeno-), Bilophila wadsworthia, Staphylococcus aureus (including MRSA), Staphyloccus epidermidis, Pseudomonas aeruginosa, Kaposi’s Sarcoma-associated herpesvirus (KSHV), Lactobacillus johnsonii, Helicobacter hepaticus, Listeria monocytogenes, Francisella tularensis (LVS strain), Mycobacterium leprae, Salmonella typhimurium, Vesicular Stomatitis Virus, Indiana-1 (VSV), Cyclosporine A, Nanoparticles, radioisotopes, MPTP, various Chemo Drugs

BSRB B60/B70 (DLAM; ABSL2/2+)

Human cells, Lenti Virus, Adeno Virus, Retro Virus, HIV-1 & -2, SIV, SHIV, HCV, Diphtheria Toxin, Viral Vectors, LCMV, Propionibacterium acnes, Human Herpesvirus-8, Cyclophosphamide, Fludarabine, MPTP, Mycobacterium Bovis (BCG vaccine strain), Klebsiella pneumoniae, Staphylococcus epidermidis, Vibrio vulnificus, Streptococcus pneumoniae, Yersinia enterocolitica, Vibrio vulnificus, Enteropathogenic Eschericia coli, AZT, other chemicals not deemed carcinogenic or toxic but where the waste must be disposed of Chem waste.

BSRB- B80A (DLAM; ABSL-1)

Used for approved chemical work with breeding mice (short term)

BSRB 246G (PI-Modlin, ABSL-2):

Mycobacterium leprae-injected zebrafish embryos

Franz Hall 288A (PI-Silva; ABSL-2

HSV-1; Modified (G-deleted) Rabies Virus; Recombinant viral vectors (lenti-, MSV-based)

Franz Hall B252-B2 (PI-Fanselow; ABSL-2)

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Franz Hall C530A (PI-Wassum; ABSL-1)

Tetrodotoxin; Conotoxin (non-SAT types)

MRL B558A (PI-Witte; ABSL-2/2+)

Human cells, Recombinant viral vectors (lenti-, retro-, adeno-)

NRB 320E/F - 320E approved for human cells and recombinant viral vector (lenti-, adeno-); 320F BDRU, Tamoxifen, 5 Fluorouracil, VCD (4-vinylcyclohexene diepoxide)

NRB 420J (PI-Carmichael; ABSL-1)

Botulinum toxin A

NRB 520 suite (DLAM; ABSL-2)

Recombinant AAV in primates

TLSB B112 (PI-White; ABSL-2):

HSV-1, Recombinant lentiviral and AAV vectors in zebra finches

TLSB B129A (PI-Edgerton; ABSL-2):

Recombinant Pseudorabies Virus (PRV), rAAV, canine adenovirus

TLSB B156B1, C (DLAM; ABSL-2)

Human cells, Recombinant viral vectors (lenti- and retro-), Carboplatin, Vorinostat, Decitabine

b) Describe circumstances and conditions where animals are housed in rooms outside of dedicated containment facilities (i.e., in standard animal holding rooms). Include practices and procedures used to ensure hazard containment.

Animals involved in studies with hazardous agents may be housed outside of dedicated containment facilities if justified and approved by the appropriate campus regulatory body or division (ARC, Institutional Biosafety Committee [IBC], ChemSafety, etc.), which certifies that sufficient SOPs have been developed to protect both laboratory and DLAM animal care staff from exposure risks. Often members of EH&S and ChemSafety work together with DLAM veterinarians and laboratory staff to develop these SOPs. The SOPs include engineering, administrative and personal protective equipment (PPE) controls tailored to both the hazard(s) and the procedures being conducted, and cover the work from receipt of the hazardous compound in the laboratory to disposal of the animal carcass. During the time period that animals are considered to be hazardous, laboratory staff are responsible for husbandry duties. Special instruction tags and stickers are placed on each cage to indicate the hazard being worked with, and the name and contact information for laboratory personnel. For example, the IBC recently approved that most adeno-associated virus (AAV) work could be performed in animals at BSL level 1 outside of dedicated containment facilities, provided that a specific, standardized SOP was followed for husbandry and animal care for the first seventy-two (72) hours following injection of the virus. This SOP, as well as others that are laboratory-specific, will be available for review at the time of

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the site visit, upon request.

c) Describe special equipment related to hazard containment; include methods, frequency, and entity(ies) responsible for assessing proper function of such equipment.

PAPR units are used to service the TB room 3V317. These are checked daily by DLAM staff to ensure proper function. An equipment service check list is used to note condition of PAPR unit when used.

Biosafety Cabinets are tested annually by a contracted service provider, TSS.

Innovive rodent racks, the monitor screen, is checked daily for proper readings by DLAM. The Innovive exhaust blowers and filters are tested annually by TSS.

The chemical fume hood located in NRB 320F is tested annually by EHS. Baulin-tubes™ and are monitored daily by DLAM staff. Eyewashes/showers tested monthly by Facilities Management (or DLAM

in the hazardous containment areas) An alarm system, which will signal a reversal of air pressure, has just

been installed in the CHS 3V TB area. We need to determine how this piece of equipment will be tested and by whom.

Sinks/handwashes are the responsibility of DLAM inside the central vivarium and the PI’s or core director’s responsibility to maintain outside the DLAM areas.

Autoclaves/cage washers/cage rack washers for any non-disposable equipment are monitored regularly (via strip tests, spore tests, RODAC plates and/or ATP testing as appropriate) and according to DLAM SOPs.

Animal transport carts (for BH pigs/NHPs) are monitored for proper function by DLAM or research staff at the time of use.

d) Describe the husbandry practices in place to ensure personnel safety, including any additional personnel protective equipment used when work assignment involves hazardous agents.

Use of PPE is mandatory within the hazardous containment facilities as instructed during training. Donning and doffing instructions are posted within each hazardous containment facility. PPE includes: gown, cap, shoe covers, double gloves, eye protection (with splash/spray risks) and appropriate mask, depending on the risk level. In some cases, respirators are required (for Tb work area or for biohazardous work performed outside the BSC). Tyvek sleeves are required when working in NHP areas.

Rodent cages are only opened under a Class II biosafety cabinet, unless approved otherwise by the IBC. Mice exposed to hazards are handled using disinfectant dipped forceps with plastic dipped tips. Disposable rodent cages

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are used to minimize handling of contaminated cages and disposed of as hazardous waste. The hazardous containment facility supervisor provides daily oversight and the DLAM Safety Officer conducts periodic inspections, including SOP review. The UCLA Biosafety Officer(s) also conduct inspections and investigations in the event of an incident, exposure, spills, or near-misses.

e) Incidental Animal Contact and Patient Areas

i) List and describe facilities that may be used for both animal- and human-based research or patient areas, including the policies and procedures for human patient protection, facility decontamination, animal transport through common corridors or elevators, and other personnel protection procedures.

Two human-based/patient areas are currently approved for animal research: 300 Medical Plaza, rooms B130F, B135H and B-165-67 (200 Medical Plaza; MRI-HIFU): MRI scanner Ahmanson (Brain Mapping), 3 rooms: MRI scanner. The ARC Policy Animal Use in Human Clinical Facilities (http://ora.research.ucla.edu/RSAWA/ARC/Pages/ARC-policies/clinical-facilities.aspx) addresses concerns relating to potential exposure of patients to animal allergens or pathogens, infection control, and potential for visibility of animal procedures by the public.

ii) Describe any other circumstances in which animals or caging equipment are transported in common use corridors or elevators (e.g., have the potential to come in contact with individuals not associated with the animal care and use program), and measures taken to mitigate risks associated with such use.

The ARC Policy, Transporting Animals in Public Access Areas and Off-Campus (http://ora.research.ucla.edu/RSAWA/ARC/Pages/ARC-policies/animal-transport.aspx ) addresses transporting animals in public access areas such as common use corridors, elevators, roadways, etc. and includes requirements for staff and vehicles to address public health, animal welfare and visibility concerns. Procedures developed according to this policy include: covered macaque carts for transport for MRI procedures; covered chair for NHPs for Bisley lab; pigs and dogs transported in solid steel transport cages, and; rabbits transported in dog carriers with covered plastic bags.

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B. Program Oversight

1. The Role of the IACUC/OB [Guide, pp. 24-40]

a. IACUC/OB Composition and Function [Guide, pp. 17; 24-25]Please provide a Committee roster, indicating names, degrees, membership role, and affiliation (e.g., Department/Division) as Appendix 7.

i. Describe Committee membership appointment procedures.

Potential committee members are recommended by current members, the ARC administrative staff, departmental personnel, and other sources. Following an initial screening by the ARC Chair, the IO is provided with a description of what role the individual will serve and why their membership should be considered. Upon approval by the IO, an invitation to serve on the ARC is extended and a new member orientation is conducted.

ii. Describe frequency of Committee meetings. Note that Appendix 8 should contain the last two IACUC/OB meeting minutes.

The ARC meets twice/month.

iii. Describe the orientation, training, and continuing education opportunities for IACUC/OB members. [Guide, p. 17]

New members complete the online CITI course, “Essentials for IACUC Members,” and participate in an orientation session with the ARC administrative staff. Topics covered in the CITI course and during the orientation include an overview of federal regulations and relevant policies/guidelines; key principles concerning humane animal care and use; the responsibilities, functions, and authority of the IACUC, Institutional Official, Attending Veterinarian, and research investigators; procedures for protocol review, approval, and post-approval monitoring; procedures for handling and reporting of animal welfare concerns; and institution-specific policies and procedures. New members are provided copies of relevant federal and state laws and regulations, guidelines, and institutional policies at the time of orientation or sent links to access these documents online.

Continuing education is provided to members through discussion and review of relevant journal articles, and updates regarding proposed changes to federal and state laws regarding the care and use of laboratory animals. Members are also provided the opportunity to view online webinars offered by OLAW and NABR and to attend relevant in-house workshops.

b. Protocol Review [Guide, pp. 25-27]A blank copy of your institution’s protocol review form should be provided as

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Appendix 9. Also include forms used for annual renewal, modifications, amendments, etc., as applicable.

i. Describe the process for reviewing and approving animal use. Include descriptions of how: the IACUC/OB weighs the potential adverse effects of the study against

the potential benefits that may result from the use (“harm-benefit analysis”),

protocols that have the potential to cause pain or distress to animals are reviewed and alternative methodologies reviewed,

veterinary input is provided, and the use of animals and experimental group sizes are justified.

Note: Make sure you address each of the items above.

The ARC utilizes the following methods for reviewing and approving animal use and associated changes: full committee review (FCR), designated member review (DMR), Chair/Vet review for significant changes allowed by OLAW/USDA (also known as VVC), and administrative/consultant review (for non-significant changes).

During FCR of applications that involve the potential for unrelieved pain or distress, the ARC performs a harm-benefit analysis. Specifically, the scientist reviewer will discuss the focus of the research and explain how the pain/distress experienced by animals in Category E does or does not outweigh the benefits of the research. This discussion is documented in the ARC meeting minutes.

Protocols that may cause more than momentary or slight pain or distress are required to include a search for alternatives. The scientist reviewer (if FCR) or DM reviewer evaluate the search strategy during their review of the protocol and make recommendations for additional searches or a consultation with the UCLA Biomedical Librarian, if appropriate.

The DLAM veterinary staff are involved in protocol review from the pre-review stage, through DMR/FCR, and in the evaluation of PI responses to committee correspondence.

With respect to justification for the use of animals, the PI must address the following question in the Rationale section of the ARC protocol form:

‘Explain the rationale for the use of animals, including (a) why the chosen species is the most appropriate for the study and (b) why the chosen species cannot be replaced with a phylogenetically lower species. Note that cost cannot be accepted as a justification.’

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With respect to the numbers justification, the ARC protocol form requests the following in the Experimental Design section:

‘Provide a complete description of: (a) all activities involving the use of research animals; (b) a scientific justification for the total number of animals required to conduct this study. The number of animals justified in this section must match the totals in the Pain Category Assignments. To the extent possible, assign all animals to experimental groups, which can be easily distinguished by the independent variables defining each group (e.g., drug dosages, time points, controls, etc.). Clearly indicate the number of animals needed per group and explain how group sizes were determined, either(i) by statistical analysis, or (ii) where statistics are not applicable (e.g., teaching labs, feasibility studies, antibody production, etc.), on the basis of other considerations (e.g., student/animal ratio, tissue yield per animal, antigen/animal ratio, prior experience, etc.). If statistical analysis is employed to determine the number of animals required, please specify the statistical method used.’

ii. Describe the process for reviewing and approving amendments, modifications, and revised protocols. If applicable, include a description/definition of “major” vs. “minor” amendments.Note: If preferred, this information may be provided in a Table or additional Appendix.

Amendments are reviewed using DMR or FCR as applicable, depending on the nature of the proposed change and the criteria the ARC has established for protocols that require FCR. Other amendments may qualify for the Chair/Vet review process described above. The ARC has approved the following: Criteria for Protocols Requiring Full Committee Review (FCR):

The following list should be used as a guide for determining whether FCR is necessary. Exceptions may be approved by the Chair or Vice Chair. A. Cats, dogs, and non-human primates, with the exception of observational studies.B. Animals listed in Pain Category E.C. Experiments that may deleteriously affect animal health, including, but not restricted to:1. Death as an endpoint / LD50-type studies 2. Prolonged physical restraint (>15 minutes) of an unanesthetized animal,3. Food and/or water deprivation >18 hours for reasons other than surgical preparation,4. Multiple major survival surgeries.D. Requested exceptions to established ARC policies. Note: Some ARC policies permit veterinary discretion for exceptions on a case-by-case basis. All other exceptions require ARC approval.

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E. Unexpected deaths not previously reported to the Committee.* The criteria described in A-D pertain to new/renewal applications and amendment/continuation applications with relevant experimental changes. These criteria do not pertain to continuation or amendment applications in which no changes related to these criteria are requested or to protocols in which research is performed entirely at another institution. E applies to all protocols.

The ARC Policy on Review of Significant Changes to Previously Approved Protocols addresses amendments that may be reviewed outside of DMR/FCR:

‘This policy is intended to clarify the process for determining what constitutes a “significant change” to an approved ARC protocol, and to describe the process for review of these activities. ARC Review of Significant Changes Review of Non-Significant Changes

IACUC approval of proposed animal activities or significant changes to previously approved animal activities is generally only granted after full committee review (FCR) or designated member review (DMR). However, thanks to new guidance from OLAW, the IACUC now has some discretion to use local policies to define what it considers a significant change, or to establish a mechanism for determining significance on a case-by-case basis in accordance with the PHS Policy IV.C.1.a.-g. According to OLAW, “…significant changes include changes that have, or have the potential to have, a negative impact on animal welfare. In addition, some activities that may not have a direct impact on animal welfare are also considered to be significant.” In an effort to reduce regulatory burden, and acknowledging the roles of professional judgment and performance standards, OLAW also allows institutions to develop policies to allow administrative handling of some significant changes. See the OLAW Guidance on Significant Changes to Animal Activities for more information. ARC Review of Significant Changes With the exceptions outlined by OLAW, the ARC must review all proposed significant changes using either the Full Committee Review (FCR) or Designated Member Review (DMR) processes (see http://ora.research.ucla.edu/OARO/Pages/applications.aspx#reviewprocess). Significant changes that must be reviewed by FCR or DMR include changes: a. from non-survival to survival surgery; b. resulting in greater pain, distress, or degree of invasiveness;c. in housing and or use of animals in a location that is not part of the animal program currently overseen by the IACUC;

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d. in species;e. in overall study objectives;f. in Principal Investigator (PI);g. that impact personnel safety. Investigators are advised to build flexibility into their protocols in order to minimize the likelihood that significant changes must be made to the protocol (e.g., including a maximum volume of blood to be collected, alternate methods of blood collection, a range of drug doses to be administered). If a proposed significant change does not appear on the above list of significant changes requiring FCR or DMR, it may be eligible for administrative review. At the discretion of the ARC Chair or Vice-Chair, the specific changes described below may be handled administratively:a. anesthesia, analgesia, sedation, or experimental substances;b. euthanasia using any method approved in the AVMA Guidelines for the Euthanasia of Animals;c. duration, frequency, type, or number of procedures performed on an animal;d. increase in previously approved animal numbers, so long as the increased number of animals requested is ≤50% of the number last approved via DMR or FCR. The ARC Chair or Vice-Chair is empowered to review an increase in previously approved animal numbers (d). Changes described under a-c above may be reviewed by the ARC Chair or Vice-Chair in consultation with the authorized veterinarian. [2] Review of Non-Significant Changes Changes that are considered not significant may be reviewed by the ARC Chair or Vice-Chair, or authorized OARO staff [3]; these changes include: a. personnel, excluding the PI;b. contact information;c. title of ARC protocol; andd. funding. In all cases, the PI must submit an amendment, in the regular manner, describing the changes for review.’

c. Special Considerations for IACUC/OB Review [Guide, pp. 5; 27-33]

i. Experimental and Humane Endpoints [Guide, pp. 27-28]

1) Describe the IACUC/OB’s review of “humane endpoints,” i.e., alternatives to experimental endpoints to prevent or in response to unrelieved animal

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pain and distress.

The ARC protocol form requires that the following question be addressed for all submissions:

Animal Care section, question #4: ‘For all types of experiments, if animals may experience complications, please describe the criteria for premature euthanasia below.’

The criteria provided in response to this question are evaluated for appropriateness based on the model and anticipated complications or side effects. The veterinary staff are generally asked to review this information, particularly for non-routine models and animals listed in pain categories D and E.

2) For studies in which humane alternative endpoints are not available, describe the IACUC/OB’s consideration of animal monitoring and other means used to minimize pain and distress (e.g., pilot studies, special monitoring, other alternatives).

The ARC requires that investigators identify criteria for premature euthanasia in the protocol. In cases where the animals are proposed to reach a moribund state or to die on their own, the Committee refers to the ARC Policy on Death as an Endpoint:

‘Policy Legal, regulatory, and moral guidelines require that animal pain, distress, and suffering be minimized in any experiment. For these reasons, investigators are required to administer euthanasia in death endpoint experiments prior to the actual death of the animals unless experimental validity will be compromised. Moreover, animals in these experiments must be monitored at least daily (including weekends and holidays) by personnel trained and experienced in recognizing signs of morbidity. More frequent monitoring may be indicated for some experimental protocols. For experiments where scientific validity requires actual death as an endpoint, the experimental design must reflect a rigorous effort to minimize the number of animals. Background Investigators must be able to judge and perform euthanasia on moribund animals based on objective signs of dying, depending on experience with the animal model, professional judgment, and the experimental protocol. Some of the known signs of illness or dying which may be applied are listed below to

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assist investigators. The specific indicators to be used for euthanasia must be included in the design of the experimental protocol. However, the particular combination of signs indicating euthanasia will vary depending on the experimental endpoints. Signs for Recognizing and Evaluating Illness, Injury, Pain, or Disease respiration very slow, very rapid, shallow, or labored rapid weight loss (such as 10% in 48 hr) and/or decrease in muscle mass or

decrease in body condition score ruffled fur (rough hair coat) hunched posture hypothermia or hyperthermia (based on measured body temperature) severe ulcerative dermatitis or infected/ulcerated tumors inappetence (may be difficult to evaluate if group housed) diarrhea or constipation (constipation may be difficult to evaluate if group

housed) impaired ambulation lethargy/inactivity/decreased normal activity muscle atrophy (decreasing muscle mass) neurologic signs including seizures, ataxia (incoordination), head tilt,

circling dehydration ocular infections/discharge, persistent squinting Strategies for Reducing Animal Numbers in Death-endpoint Experiments The traditional LD50 experiment to measure toxicity is widely criticized as cruel and wasteful of animals. This procedure involves groups of animals that are exposed to increasing doses of a toxic substance or infectious agent to determine the dose required to kill 50% of the animals. Because of the relatively large numbers of experimental animals involved, use of the LD50 is no longer considered acceptable by federal regulatory agencies. As reviewed in the references below, statistical methods have been developed that reduce the number of vertebrate animals used in experiments without compromising experimental reliability. One approach that has been used to derive median values with relatively few samples is the up-and-down procedure. Whereas conventional methods using a dose-response experimental design generally employ 24 to 40 subjects, LD50 values calculated through the up-and-down procedure can use as few as six animals. The up-and-down procedure yields essentially identical LD50 values as the conventional dose-response experiments. Those investigators whose work requires death as an

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endpoint must review current statistical approaches to reducing animal numbers and apply these methods whenever possible.’

3) Identify personnel responsible for monitoring animals for potential pain and distress and describe any mechanisms in place to ensure that the personnel have received appropriate species- and study-specific training.

All laboratory personnel that will handle animals, including those that monitor animals for signs of pain and/or distress, are required to be listed as personnel on a protocol. At a minimum the ARC requires completion of the CITI online “Animal Research” training and species-specific training prior to approving personnel to work in a lab.

ii. Unexpected Outcomes that Affect Animal Well-being [Guide, pp. 28-29]Describe how unexpected outcomes of experimental procedures (e.g., unexpected morbidity or mortality, unanticipated phenotypes in genetically-modified animals) are identified, interpreted, and reported to the IACUC/OB.

Unexpected outcomes, including unexpected morbidity or mortality, are reported to the ARC by the PI, research personnel, and/or the DLAM veterinary staff, and this may be done in the context of an annual or triennial review or via a separate report. In the case of the former, these reports are reviewed as part of the application and additional information requested, if appropriate. If the latter, the report is reviewed by a subcommittee of the ARC Chair and AV to determine if additional information is needed and/or if the report should be forwarded to the ARC for further review.

iii. Physical Restraint [Guide, pp. 29-30]Note: This section is to include only those protocols that require prolonged restraint. Brief restraint for the purpose of performing routine clinical or experimental procedures need not be described.

1) Briefly describe the policies for the use of physical restraint procedures or devices. Include, if applicable, the IACUC/OB definition of “prolonged.”

An excerpt from the ARC Policy on Physical Restraint of Unanesthetized Animals is as follows:

‘Physical Restraint of Unanesthetized Animals

Prolonged physical restraint should be avoided unless essential to the research objectives. All physical restraint, other than routine manual restraint, must be described in the protocol. Physical restraint for periods longer than 15 minutes must be described in detail and justified for approval by the Animal Research Committee (ARC). Convenience is not justification to use prolonged physical

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restraint. The least restrictive method of restraint possible should be used, even though it may be more costly and technically more difficult. When prolonged physical restraint is required, the following considerations must be addressed: 1. Once a protocol involving prolonged physical restraint has been approved by the ARC, the animals undergoing prolonged physical restraint must be observed by a member of the Division of Laboratory Animal Medicine (DLAM) veterinary staff during the initial conduct of the experiment to ensure that the animals are not undergoing undue distress. 2. Unless an exception has been specifically approved in the animal use protocol, animals to be placed in restraining equipment should be conditioned to the equipment by gradually increasing time of restraint until the required restraint time is reached. 3. The period of restraint must be limited to the minimum required to accomplish the research objectives. 4. For the comfort and safety of the animal, certain types of restraint equipment, such as slings for dogs, require that the animals be attended continuously throughout the period of restraint. For each situation, the ARC will make a determination as to the intensity of the attention required. 5. Nonhuman primates must not be maintained in restraint devices unless required for health reasons as determined by the Attending Veterinarian or as part of a research proposal approved by the Committee. Maintenance under such restraint must be for the shortest period possible. 6. Attention must be given to the possible development of lesions or illnesses associated with restraint, including contusions, decubital ulcers, dependent edema, and weight loss. If these or other problems occur, prompt veterinary care must be provided. If the DLAM veterinarian tending the animal considers the health problem serious, the well-being of the animal must take priority over the experimental objectives.’

2) Describe animal restraint devices that are used or have been used within the last three years. For each device, briefly describe the duration of confinement acclimation procedures monitoring procedures criteria for removing animals that do not adapt or acclimate, and provision of veterinary care for animals with adverse clinical

consequences.

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Note: If preferred, this information may be provided in a Table or additional Appendix.

Information on restraint devices used within the last three years is provided in Appendix 21, which lists: the protocol number:, species used, rationale for restraint, type of device, conditioning of the animal, restraint duration and frequency, and monitoring during the restraint period. We do not specifically ask for criteria for removing animals that do not adapt or acclimate on the ARC protocol, therefore that information is not readily available for a report. Regarding provision of veterinary care for animals with adverse clinical consequences, those cases would be routed through our regular process for reporting and addressing animal health concerns.

iv. Multiple Survival Surgical Procedures [Guide, p. 30]Note: One survival surgical procedure followed by a non-survival procedure is not included in this category.

1) Describe the IACUC/OB’s expectations regarding multiple survival surgery (major or minor) on a single animal.

The ARC requires scientific justification for performing multiple survival surgeries on a single animal. Multiple survival surgeries will be approved only when they are related components of the experimental design.

From the ARC Policy on Multiple Survival Surgeries:

‘ARC Policy Multiple survival surgeries on a single animal may be permitted only if scientifically justified by the investigator and approved by the ARC. The number of survival surgeries performed must be limited to the minimum number necessary to achieve the research objectives and must be determined with due consideration for minimizing the pain and distress experienced by any one animal. Whenever possible, all operative procedures should be done at one time to minimize post-operative discomfort and distress to the animal. Cost or convenience is not considered to be adequate justification for the conduct of multiple survival surgeries. Emergency multiple surgeries may be done to correct complications due to previous surgical procedures or as part of the process of providing veterinary care; however, these must be done in consultation with a DLAM veterinarian. Euthanasia should be considered as a humane alternative to surgical repair in

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these cases if the animal is in poor health or suffering pain or distress that cannot be alleviated. Some procedures characterized as minor may induce substantial post procedural pain or impairment and should similarly be scientifically justified if performed more than once in a single animal.’

2) Summarize the types of protocols currently approved that involve multiple major survival surgical procedures

Note: If preferred, this information may be provided in a Table or additional Appendix.

A list of protocols currently approved for multiple major survival surgeries is provided in Appendix 22 and lists PI name, protocol number, species by number approved and pain category.

v. Food and Fluid Regulation [Guide, pp. 30-31]. Note: This does not include pre-surgical fast.

Summarize the types of protocols that require food and/or fluid regulation or restriction, including:

justification species involved length and type of food/fluid regulation animal health monitoring procedures and frequency (e.g., body

weight, blood urea nitrogen, urine/fecal output, food/fluid consumption)

methods of ensuring adequate nutrition and hydration during the regulated period

Note: If preferred, this information may be provided in a Table or additional Appendix.

Current protocols that include food and/or fluid restriction (other than that required pre-surgery) are included in Appendix 23 and lists: protocol number, and details of the food or fluid restriction.

vi. Use of Non-Pharmaceutical-Grade Drugs and Other Substances [Guide, p. 31]Describe the IACUC/OB’s expectations regarding the justification for using non-pharmaceutical-grade drugs or other substances, if applicable.

An excerpt from the ARC Policy on Use of Pharmaceutical-Grade Compounds is as follows:

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‘In accordance with the NIH Office of Laboratory Animal Welfare, USDA Animal Care Policy # 3, and the Guide for the Care and Use of Laboratory Animals (the Guide, 8th edition, p. 31), the Animal Research Committee (ARC) has established the following guidelines:Unless approved by the ARC, investigators are expected to use pharmaceutical-grade or veterinary grade medications, anesthetics, analgesics, euthanasia agents and experimental agents whenever they are available, even in acute procedures. Investigators should consider relevant animal welfare and scientific issues

including safety, efficacy, and the inadvertent introduction of new variables when using non-pharmaceutical grade compounds.

Use of non-pharmaceutical grade/veterinary grade agents must be justified in the protocol and submitted to the ARC for specific review and approval. Anesthetics, analgesics and sedatives used to treat more than momentary or slight pain or distress, and euthanasia agents, must be pharmaceutical/veterinary grade unless used as investigational agents. Examples of acceptable justification for use of non-pharmaceutical/veterinary grade investigational agents include: 1) the compound is not available in a pharmaceutical-grade preparation and comparable alternative agents available in pharmaceutical grade form cannot be used for scientific reasons; 2) it is necessary to compare data with previous experiments using the non-pharmaceutical grade substance; 3) it would be necessary to dilute the pharmaceutical grade preparation thereby compromising the pharmaceutical grade quality of the preparation; 4) the vehicle of the pharmaceutical grade preparation cannot be determined preventing use of an appropriate control.

Cost savings alone is not an adequate justification for using non-pharmaceutical-grade compounds in animals.

All non-pharmaceutical- and/or veterinary-grade compounds and diluents must be sterilized (e.g. autoclaved or filter-sterilized using a 0.22 µm filter prior to administration) wherever this is possible without jeopardizing the activity/stability of the agent.’

vii. Field Investigations [Guide, p. 32]Describe any additional considerations used by the IACUC/OB when reviewing field investigations of animals (non-domesticated vertebrate species), if applicable.

During the administrative pre-review of field study protocols, PIs are asked to identify and provide all permits required to perform the work (if permits to not identify allowed activities, a copy of the permit application is also requested), as well as consult with the OHF Medical Director, T. Warner Hudson to discuss risks associated with the research. Prior to ARC approval of the protocol, the ARC administrative staff will verify that the above have been completed.

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In addition, the Guidelines of the American Society of Mammalogists for the Use of Wild Mammals in Research are available for use during review of field studies.

viii. Animal Reuse [Guide, p. 5]1) Describe institutional policies regarding, and oversight of, animal reuse

(i.e., on multiple teaching or research protocols).

The ARC protocol indicates the final disposition of all animals; if animals are not euthanized at the end of a study, their final disposition, including transfer to another protocol or study, is indicated. This would also include donation to the DLAM teaching animal colonies (mice, rats, rabbits). During protocol review, if pain category C animals are identified that are not needed at the end of a study for tissue collection, the vet may suggest that these be donated to DLAM for training or offered for use by another investigator. In the event that a PI requests to reuse animals (e.g., for ongoing behavioral testing following training), the ARC considers the well-being of the animals and whether the reduction in total animals used warrants the continued use of an animal.

2) Briefly describe the types of activities currently approved that involve the reuse of individual animals.Note: A list of specific protocols involving reuse of animals should be available during the site visit.

ARC #2002-064 (Species: Pigeon)When possible, pigeons that had served as subjects in previous experiments will be reused in subsequent experiments. Pigeons typically live for more than 15 years in captivity. We reuse our subjects in experiments throughout their lifetime (barring injury or illness) so that a typical subject will participate in dozens of experiments during its tenure in our laboratory. Individuals not actively involved in an experiment remain in the colony on this protocol until they are assigned to an experiment. After completing an experiment, a pigeon will be reassigned to a new experiment anywhere from immediately to a few months after the experiment is completed. Animals are not transferred to other labs or protocols.

ARC #2006-023 (Species: NHP)Generally, two animals are involved in a particular experiment, so we would expect to use 12 animals. However, as in the last 3 year period, monkeys will participate in multiple experiments. Each monkey usually works on a study for 4-24 months. Once that study is completed, we then use the same monkey, usually performing the same behavioral task, for a new experiment. As such a monkey who starts off as a behavioral monkey, may then join a single unit recording experiment, or a monkey who starts off in a recording experiment may then go on to a microstimulation experiment, etc. Thus, we expect that each animal will be a part of one or two experiments over the next 3 year

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period; so we expect to use 8 animals.We feel it is ethically more justifiable to use the same few subjects repeatedly, especially once they are trained on complex behavioral tasks and used to the water schedule protocol, rather than using new subjects for each experiment. I expect that a significant number of the monkeys used in this protocol will continue into future renewals, just as we have kept 2 animals from the last 3-year cycle (indeed, they were brought in two protocol cycles ago). This is one of the ways that we attempt to use the fewest total number of animals as possible in the long run.

ARC #2012-043 (Species: NHP)We are requesting a total of 15 animals for a three year period. In all likelihood we will not use that many because we routinely use well-trained animals in different behavioral experiments combined with electrophysiology. We believe it is ethically more justifiable to use the same few subjects repeatedly, especially once they are trained on complex behavioral tasks and used to the water schedule protocol, rather than using new subjects for each experiment. We expect that a significant number of the monkeys used in this protocol will continue into future renewals as they have for this renewal. In net for this current renewal, we plan for up to 9 animals for the electrophysiological experiments (but if all experiments lead to similar results between two monkeys then we will only need 6), 6 for the optogenetics and fMRI experiments and 2 for the Parkinson’s disease experiments and 12 for the motor nerve degeneration experiments. If we used naïve animals for each of these experiments that would require 29 animals. However since we will use the same animals for different aspects of different experiments we are requesting only 15. The same 9 will be used for ephys and the motor nerve studies, and the same animals will be used for optogenetics and fMRI and ephys (the optogenetics and fMRI experiment will occur first to ensure they are naïve at that time). Only 2 will be used short term for the Parkinson’s experiments and will not also participate in any other experiments, unless the first animal is very successful then we may try to collect electrophysiological data in the Parkinson’s animal for preliminary data for a new Udall application.

ARC #2004-064 (Species: Fish, Salamander, Toad)Live animals provide invaluable opportunity for students to gain understanding of various vertebrate species by observing their morphology, behaviors and their simulated habitats. The knowledge and appreciation obtained through live demonstration cannot be replaced by preserved specimens. The animals will be kept alive and healthy for repeated use in observation by LS1 students.

ARC #1998-159 (Species: Fish)At the end of an exercise the fish will be placed back to their original tank and allowed to recover for at least three hours during the next lab section. Students of the next lab section will use fish from an alternate fish holding tank. In

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summary each fish gets exposed about 5 times per quarter to each of the randomly chosen five parameters. The goldfish do not get euthanized by the experiment and are kept through the reminder of the quarter to be reused next quarter. When a fish becomes too large for the experimental chamber and/or the capacity of the holding tank, it is donated to the outdoor pond of a local school (to be approved through Fish & Game/CDFA and ARC prior to release).

ARC #2001-191 (Species: Marmot)Please note that animals are studied throughout their lives and we make many measurements and conduct many observations on them throughout their lives. Thus, formally, animals are re-used for different studies, hence the total number of animals studied is estimated at 400 per year.

ARC #1999-169 (Species: Multiple)This is the DLAM training protocol for rodents (mice, rats, gerbils, hamsters and Guinea pigs). At the end of their usefulness for training purposes (as defined by the protocol), animals may be euthanized, transferred to other ARC-approved protocols with PIs at UCLA, adopted by a DLAM staff member, or transferred to other similar protocols at other institutions for training purposes. Note that no animals that will have undergone surgical procedures will be transferred to other protocols; it will only be animals that have undergone simple handling, aseptic surgical prep, or basic non-surgical procedures, such as injections, blood collections, etc., that would be transferred to other protocols (either at UCLA or other institutions) for further use. Animals that would be adopted may be post-operative but would be in good health as determined by DLAM veterinary exam.

ARC#2003-044 (Species: Mouse)This is the DLAM rederivation protocol. Females that are not selected as embryo transfer recipients will be transferred to the DLAM training protocol. Females that were embryo recipients (via surgical or non-surgical embryo transfer) and do not bear a litter are also transferred to the DLAM training protocol. The surgical history of those females will follow them to the training program and they will not be used for any surgical training procedures.

ARC#2013-074 (Species: Rabbit)This is the DLAM training protocol for rabbits. Animals that have not undergone surgical procedures may be transferred to other ARC approved protocols.

ARC#2014-066 (Species: Dog)This is DLAM’s training protocol for dogs and pigs. Dogs that are not euthanized at the end of the training session (which includes non-survival surgery on this protocol) may be adopted out.

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3) Describe other instances where the final disposition of animals following study does not involve euthanasia, including adoption, re-homing, rehabilitation, etc. Note: A list of specific protocols involving reuse of animals should be available during the site visit.

In most cases, animals are euthanized at the end of the study. Field studies in which animals are captured and sampled generally involve release as opposed to euthanasia.

ARC #2011-060 (Species: Gerbil, Hamster, Mouse, Rat)For uninfected animals, adoption will used as an alternative to euthanasia when possible.

ARC #2015-052 (Species: Mole, Mouse, Rat, Shrew, Vole)They will be re-released. Animals will not be euthanized unless injured.

ARC #2013-001 (Species: Agouti, Amphibians, Bird, Fish, Lizard)These animals will be released to the wild once marked, in the rare case in which an animal is judged to be injured by trapping/handling beyond the point where it could survive in the wild, the animal would be euthanized. We will not be handling or coming within 15 m of any birds that we study. No euthanasia is necessary.

ARC #2012-030 (Species: Rat)Dams will be saved for continuing breeding. For animals losing breeding ability, they will be donated to DLAM or euthanized following DLAM protocol.

ARC #2008-033 (Species: Bird)ARC #2007-001 (Species: Bird)All individuals are released alive at point of capture back into the wild. Birds are released back to the wild after approximately 15 minutes of handling.

ARC #2001-191 (Species: Marmot)All work with living animals will be conducted at the Rocky Mountain Biological Laboratory, Gothic, Colorado. We are conducting many simultaneous studies with this free-living population; most of them are minimally-invasive. The Colorado Division of Wildlife fully approves our project and issues an annual permit to trap, mark, and release animals and to salvage dead animals we find (on the road, in the field). The experimental protocol does not require euthanasia.

ARC #1992-057 (Species: Tortoise)This is a federally protected Threatened Species being studied in its natural

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habitat. Our Fish and Wildlife permit does not authorize euthanasia. Study animals are released after measurements or other procedures are completed during their temporary captivity.

ARC #2014-116 (Species: Bat)Because bats are being bred, conditioned, or held for use in teaching, testing, experiments, research, or surgery but not yet used for such purposes, they are considered USDA Category B. Prior to use in research activities (including euthanasia for tissue collection), animals will be transferred from this holding protocol to an approved research protocol using the DLAM Procurement Portal.

ARC #2012-035 (Species: Fox, Mouse, Raccoon, Rat, Sea Lion, Skunk, Squirrel, Vole)Animals will be released back into the area from which they were captured.

ARC #2012-011 (Species: Bird)Individuals will be released alive and unharmed back into the wild at the site of capture.

ARC #2010-107 (Species: Bat)Egyptian fruit bats used for behavioral tests will be maintained in our colony until they die of natural causes.

ARC #2009-123 (Species: Bird)At the end of our experiments that involve keeping birds in captivity with or without treatment with steroids, the birds are healthy and are released back into the wild. We have recaptured birds experiencing these treatments have been recaptured years later so we are confident they are healthy and can survive in the wild. Most of our birds are released.

ARC #2009-090 (Species: Zebra)Animals will remain in the wild.

ARC #2007-162 (Species: Bird)All individuals will be released alive back to the wild.

ARC #1999-169 (Species: Multiple)This is the DLAM training protocol for rodents (mice, rats, gerbils, hamsters and Guinea pigs). At the end of their usefulness for training purposes (as defined by the protocol), animals may be euthanized, transferred to other ARC-approved protocols with PIs at UCLA, adopted by a DLAM staff member, or transferred to other similar protocols at other institutions for training purposes. Note that no animals that will have undergone surgical procedures will be transferred to other protocols; it will only be animals that have undergone simple handling, aseptic surgical prep, or basic non-surgical procedures, such as

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injections, blood collections, etc., that would be transferred to other protocols (either at UCLA or other institutions) for further use. Animals that would be adopted may be post-operative but would be in good health as determined by DLAM veterinary exam.

ARC#2014-066 (Species: Dog)This is DLAM’s training protocol for dogs and pigs. Dogs that are not euthanized at the end of the training session (which includes non-survival surgery on this protocol) may be adopted out.

2. Post-Approval Monitoring [Guide, pp. 33-34]

a. Describe mechanisms for IACUC/OB review of ongoing studies and periodic proposal/protocol reviews (e.g., annual, biennial, triennial, or other frequency).

The ARC performs annual review of all protocols that use USDA-regulated species, as well as those protocols funded by DOD. All experimental protocols are subject to a 3-year de novo review. Breeding protocols are re-reviewed every 3 years.

b. Describe the process and frequency with which the IACUC/OB reviews the program of animal care and use.

As required by the PHS Policy and the Animal Welfare Regulations, the ARC reviews the program of animal care and use every six months, using the Sample OLAW Program and Facility Review Checklist.

c. Describe the process and frequency with which the IACUC/OB conducts facility and laboratory inspections. Describe the rationale or criteria used for exempting or varying the frequency

of reviewing satellite holding facilities and/or animal use areas. If contract facilities or contractor-provided personnel are used, describe

procedures used by the IACUC/OB to review such programs and facilities.Note: A copy of the last report of these reviews should be included as Appendix 10.

At least once every six months, the ARC visits all of the DLAM-maintained vivaria including animal holding areas, animal care support areas, storage areas, and procedure areas, as well as research study areas in which USDA-regulated species are used, and where animal surgeries are conducted (including those conducted on non-USDA-regulated species). Equipment used for transporting of the animals is also inspected. The ARC also has purview over all other areas where non-USDA regulated animals are used for short-term, non-surgical procedures, such as blood collection, behavioral testing, and euthanasia; those areas are inspected on a regular basis of no less than once every 24 months, as discussed with OLAW and described in our OLAW Assurance

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Statement. The Committee uses the Guide and other pertinent resources (e.g., the PHS Policy, the Animal Welfare Regulations) as a basis for the review. To facilitate the evaluation, the Committee uses a checklist based on the Sample OLAW Program and Facility Review Checklist. If deficiencies are noted during the inspection, they are categorized as significant or minor and the Committee develops a reasonable and specific plan and schedule for correcting each deficiency. A significant deficiency is one that is or may be a threat to the health and safety of the animals or personnel. No member is involuntarily excluded from participating in any portion of the inspections.

Animal work performed by contract facilities is reviewed by the ARC as follows: the PI maintains a protocol in the RATS database and submits a copy of the approved protocol and approval notice from the contractor’s IACUC for review. The ARC confirms that the contractor is registered with the USDA (when applicable), holds a PHS Animal Welfare Assurance, and is AAALAC-accredited. In cases where the contractor is not accredited, justification for use of that vendor is requested.

d. If applicable, summarize deficiencies noted during external regulatory inspections within the past three years (e.g., funding agencies, government, or other regulatory agencies) and describe institutional responses to those deficiencies. Note: Copies of all such inspection reports (if available) should be available for review by the site visitors.

No OLAW site visits during the past 3 years.USDA inspections:9/30/2014 – No non-compliant items identified during this inspection.9/29/2015 – Citations were 2.31(d)(1)(ix), 3.125(a), and 3.131(c). Please refer to the inspection report for more information.3/14/2016 – No non-compliant items identified during this inspection. This was a focused inspection.5/25/2016 – No non-compliant items identified during this inspection.9/14/2016 – No non-compliant items identified during this inspection. This was a focused inspection in response to an item under review noted on the March 14, 2016 focused inspection report.

e. Describe any other monitoring mechanisms or procedures used to facilitate ongoing protocol assessment and compliance, if applicable.

The process of protocol monitoring includes, among other activities, observations of ongoing animal procedures, a walk-through of the research facilities, discussions with the Principal Investigator (PI) and research staff, and the review of protocols and protocol related documents including charts/animal records.

Monitoring visits may be conducted by the ARC Animal Welfare Coordinator, who may be assisted by other individuals who are knowledgeable in specific technical, scientific or safety areas that are particularly relevant to the conduct of a particular

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study (e.g., individuals with microbiological or environmental health and safety expertise).

Monitoring visits may be random (not-for-cause) or targeted (for-cause) visits. Not-for-cause monitoring visits will be announced and scheduled with the PI orstudy staff in advance; for-cause monitoring visits may or may not be announced, depending on the reason for the visit, the urgency involved, and other surrounding circumstances. For-cause monitoring visits will be conducted when deemed necessary by the ARC (visits may be done by ARC staff along with ARC members, and/or vet care staff). In addition, during weekly visits to the study areas by DLAM staff, non-compliance issues may be noted and relayed to the ARC.

The PAM Program is intended to be educational (as opposed to investigatory) in nature, and is aimed at prevention (rather than punishment) to themaximum extent possible, consistent with regulatory and institutional reporting and enforcement obligations.

3. Investigating and Reporting Animal Welfare Concerns [Guide, pp. 23-24]Describe institutional methods for reporting and investigating animal welfare concerns.

An excerpt from the ARC Policy on Reporting Allegations of Mistreatment or Other Noncompliance Issues is as follows:

‘Definitions

Mistreatment: Any action, physical or psychological, which results in wrongful or abusive treatment of an animal.

Noncompliance: Violation of University policy or noncompliance with the Public Health Service Policy on Humane Care and Use of Laboratory Animals (PHS Policy), the USDA Animal Welfare Act Regulations (USDA AWAR), and other applicable federal, state, and local laws or regulations governing animal care and use.

Who May Report

Any person, including any University employee, student, volunteer, or member of the general public, may report concerns involving the care and use of animals at UCLA. Such concerns may be reported anonymously. If the complainant identifies him/herself, protection of his/her identity will be maintained to the extent possible within the legitimate needs of law and the investigation.

When and What to Report

Based on federal requirements, the ARC has identified several kinds of reportable

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incidents that may serve as examples to guide individuals in making their determinations. These incidents include, but are not limited to, the following: a condition that is or may be a threat to the health or safety of animals; the conduct of animal-related activities or protocol modifications without prior ARC review and approval; continuing activities past the protocol expiration date; the conduct of activities by uncertified and/or unlisted personnel; continuing noncompliance.

If you believe that mistreatment or noncompliance has occurred, timely reporting is essential to protect the animals involved and to facilitate the investigation of the allegations. Owing to the great diversity of potential problems, it is not possible to anticipate all of the incidents that may occur and provide an exhaustive listing of those considered reportable. As such, determination that a problem falls within the letter or spirit of either "mistreatment" or "noncompliance" requires a degree of judgment. Frequently, the attending veterinarian, animal care personnel, and investigators can work together to prevent or resolve a problem. If in doubt, it is better to submit a report, as this may well protect the institution, the complainant, the alleged violator(s) and, of course, the animals.

How to Report

Reports are encouraged to be made in writing so as to assure a clear understanding of the issues raised, but may be made verbally. Such reports should contain as much specific, factual information as possible to allow for a full investigation and proper assessment of the nature, extent, and urgency of the concern. Information should include, but need not be limited to, the nature, date, time, and location of the occurrence; the person(s) against whom the allegation is being made; and any supporting documentation.

Whom to Contact

To ensure prompt attention to any reported allegation, as well as to ensure anonymity of any "whistleblower" reports, please contact the Office of Animal Research Oversight (OARO), Institutional Official, Attending Veterinarian or veterinary staff, ARC Chairman, any ARC member, or the UCLA Compliance Office:

OARO: UCLA Compliance Office:Phone: (310) 206-6308 Hotline: (800) 403-4744Fax: (310) 206-0742 File a report online at: Email: oaro@research.ucla.edu universityofcalifornia.edu/hotlineMailing Address:UCLA Office of Animal Research Oversight Box 951694Los Angeles, CA 90095-1694

For information on investigative procedures, please refer to the ARC Policy on Investigating Allegations of Mistreatment or Other Noncompliance Issues.’

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An excerpt from the ARC Policy on Investigating Allegations of Mistreatment or Other Noncompliance Issues is as follows:

‘Initial Evaluation and Actions

Upon receipt of a reported concern, the ARC Chair, in consultation with the Campus Veterinarian, shall take immediate steps to ameliorate the problem and protect the animals. Such ameliorative steps may range from veterinary medical intervention, confiscation of the animals, and/or cessation of activities, to taking no action other than the investigation of the concern. In some cases, involvement by the Institutional Official (IO), legal counsel, and other University officials (e.g., Department Chair) may be required at the outset of the investigation.

In every investigation, the person(s) against whom the complaint has been raised shall be given notice of the concern and is provided an opportunity to address the allegations in writing. In addition, if the identity of the reporting party is known, an acknowledgment of receipt shall be given, with an assurance that an investigation is underway.

Following the initial investigation, the ARC Chair shall elect to either immediately bring the matter as a whole before the Committee or appoint a Sub-Committee to investigate the allegation. As much information as is reasonably needed will be collected, which may entail review of documents, inspection of the facilities, and/or discussions with pertinent individuals.

ARC Evaluation

Results of the initial evaluation, including all supporting documentation, will be provided to the Committee for consideration at a convened meeting. Based on the information, the ARC will determine 1) the nature of the concern as it relates to the USDA Animal Welfare Act and Regulations (AWAR), Public Health Service (PHS) Policy on Humane Care and Use of Laboratory Animals (PHS Policy), and University policy; 2) the need for additional actions, such as further investigation or notification of other University officials as appropriate; and 3) corrective measures to address the concern and prevent recurrence. In all cases, the person(s) against whom the allegations have been directed will be notified of the ARC's decisions in writing.

If the identity of the complainant is known, he/she will be notified in writing of the completion of the investigation, with an assurance that appropriate remedial action has been taken as applicable.

Confidentiality

Details pertaining to an investigation in progress remain confidential to the extent possible to protect all concerned; however, when the ARC releases the final report of its findings to

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federal regulatory agencies, those reports may become accessible to the public under the Freedom of Information Act.

For information on reporting procedures, please refer to the ARC Policy on Reporting Allegations of Mistreatment or Other Noncompliance Issues.’

4. Disaster Planning and Emergency Preparedness [Guide p. 35]Briefly describe the plan for responding to a disaster potentially impacting the animal care and use program: Identify those institutional components and personnel which would participate in

the response. Briefly describe provisions for addressing animal needs and minimizing impact to

animal welfare.Note: A copy of disaster plan(s) impacting the animal care and use program must be available for review by the site visitors.

The DLAM Emergency Response and Continuity Plan was developed in coordination with emergency planning staff in the DGSOM Office of the Dean, and complements the UCLA Emergency Response Plan developed by the Office of Environmental Health and Safety for the Emergency Management Team (EMT). The operation of the EMT is based upon the Incident Command System and is responsible for response to emergencies on a campus-wide level. The DLAM Emergency Response and Continuity Plan is site specific and covers all DLAM-managed facilities. The DLAM Emergency Response Team is composed of the AV and veterinarians, Director of Operations and other management and supervisory staff who will work with emergency response personnel in the DGSOM and EH&S in an actual event. All departments in the DGSOM are required to have a similar Emergency Response and Recover Plan; therefore most of UCLA’s animal Study Areas would be covered by one of these plans. The ARC provides all Study Areas with a similar Animal Disaster Plan which can be used if no other plan is available and refers to the DLAM Plan (e.g. for euthanasia assistance). The AV is responsible for all animals on campus and the DLAM team provides animal support wherever necessary in the event of an emergency or disaster.

The plans were developed to protect the safety of staff, visitors, and students; safeguard resources (e.g. animals, records, etc.) related to the campus’ mission; coordinate unit-level emergency preparedness and response; and, to ensure business continuity after an event.

The plan includes: Inventory and storage of hazardous material. Critical equipment location and inventory list (e.g. water, food, caging supplies,

euthanasia agents and supplies) Appropriate emergency information and training (including drills) for division

personnel. Secure storage locations for division first aid and emergency supplies Effective emergency communication

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Disaster information reporting, notification and situational status updates protocols Evacuation routes to building assembly areas. Pre-defined recall procedures for essential personnel. Strategies for relocation, treatment, or euthanasia of animals. Strategies for resuming normal operations. Advance planning for documenting and emergency’s impact and cost Emergency procurement Access for emergency personnel to all division areas.

Guidelines are provided for preparation for and response to the following types of emergencies: Accident or major medical emergency Power outage Fire Hazmat, local or area wide Flooding Earthquake Bomb threat Suspicious package Workplace violence/animal activism Other utilities failures (e.g. HVAC) Animal surgery room emergency Extreme weather

II. Animal Environment, Housing and ManagementNote: Complete each section including, where applicable, procedures performed in farm settings, field studies, aquatic environments, etc.

A. Animal EnvironmentNote: Facility-specific details regarding mechanical system construction and operation is requested in Section IV.B.5. and Appendix 11; current (measured within the last 12 months), detailed (by room) performance data must also be provided as indicated in Appendix 11.

1. Temperature and Humidity [Guide, pp. 43-45]

a. Describe the methods and frequencies of assessing, monitoring, and documenting that animal room or housing area temperature and humidity is appropriate for each species.Note: If preferred, this information may be provided in a Table or additional Appendix.

Assigned DLAM technical staff observe room temperature and humidity information from the environmental monitoring devices located in each animal holding room and

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record data on individual room maintenance logs (Room Status Sheet) daily. Room temperature and humidity reports including Hi-Low readings are sent to the area supervisor (or to the PI in study areas) daily, weekly and monthly; this data is also maintained on a Cloud server. The room temperature and humidity are monitored 24/7 by the (Sensoscientific) environmental monitoring devices, which are installed in all animal holding rooms. If room temperature/humidity vary outside acceptable ranges defined by the Guide, alarm notifications are sent via email and/or text messages to DLAM on-call staff (or to the PI in study areas) to investigate and, if necessary, report the problem to Facility Management Trouble Call Desk (staffed 24/7) during working hours as well as after regular working hours/weekends and holidays. This process is captured in DLAM’s Environmental Monitoring SOP. Samples of daily, weekly and monthly temp/hum reports will be available for review at the time of the site visit, upon request.

b. List, by species, set-points and daily fluctuations considered acceptable for animal holding room temperature and relative humidity. Note: If preferred, this information may be provided in a Table or additional Appendix. [Guide, pp. 44 and 139-140]

TemperatureSPECIES SET POINTS RANGESMice, rats 73°F 68° to 79° FRabbits 67° F 61° to 72° FPigs (indoor housing) 71° F 61° to 81° FPigs (outdoor housing) N/A*Dogs 74° F 64° to 84° FGeckos - DLAM-managed 81° F 72° to 90° F RTGeckos – Study Area 73° F 68° to 79° F RTFrogs (Xenopus, Rana) 66° F 60° to 72° F RTChinchillas 72° F 65° to 80° FNon-human primates 74° F 64° to 84° FGerbils 73° F 68° to 79° FHamsters 73° F 68° to 79° FPigeons 72° F 64° to 79° FGuinea Pigs 73° F 68° to 79° FLamprey 62° F 55° to 68° F RTChickens (as chicks) 77° F 72° to 82° F RTFish (Zebrafish) 80° F 72° to 89° F RTFish (other spp). 73° F 68° to 79° F RTSalamanders 73° F 68° to 79° F RTToads 73° F 68° to 79° F RTAxolotls 73° F 68° to 79° F RTNewts 73° F 68° to 79° F RTBirds (finches) DLAM-managed 75° F 68° to 82° F Study Area 67° F 50° to 85° F

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Bats 75° F 60° to 90° F

RT = room temperature; localized temperatures around the animals may vary, due to micro-environmental factors (such as heat lamps, heat rocks, aquatic species in tanks, etc.).*For pigs in the outdoor runs, there is no set point as the temperature will be whatever the ambient temperature is outside: heaters provided for this area turn on at 61° F and at 81° F, the misters are turned on or pigs are moved indoors.

HumiditySPECIES RANGESMice, rats 30 – 70%Rabbits 30 – 70%Pigs (indoor housing) 30 – 70%Pigs (outdoor housing) ambientDogs 30 – 70%Geckos 30 – 70% RHFrogs (Xenopus, Rana) none – 98% **Chinchillas 30 – 50%Non-human primates 30 – 70%Gerbils 30 – 70%Hamsters 30 – 70%Pigeons 30 – 70%Guinea Pigs 30 – 70%Lamprey none – 98% **Chickens (as chicks) 30 – 70%Fish none – 98% **Salamanders 30 – 70% RHToads 30 – 70% RHAxolotls none – 98% **Newts none – 98% **Birds (finches) 30 – 70%Bats 40 – 80%

RH = room humidity; humidity in the enclosures may be increased due to the presence of intra-enclosure devices such as water-bowls, automatic water sprayers, and other materials to increase relative humidity. Refer to species-specific SOPs for details.

**For aquatic areas, the ARC has widened the range; an upper limit of 98% was set to help prevent condensation on tanks; no lower limit was set. Refer to ARC Study Area Policy: Maintaining Animals in Study Areas http://ora.research.ucla.edu/RSAWA/ARC/Pages/ARC-policies/study-areas.aspx .

For temperature, fluctuations of +/- 3°F are tolerated (although if temperatures stay at the low or high end of this range, a non-urgent request will be sent to Facilities Management to address the issue so the room temperature will be returned to the set

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point). Anything outside of the ranges provided in the table above will send an immediate alert to DLAM staff or the PI (in study areas) who will contact Facilities Management who will immediately address the issue.

c. Temperature set-points in animal housing rooms and/or environmental conditions are often outside of the species-specific thermoneutral zone. Describe the process for enabling behavioral thermoregulation (e.g., nesting material, shelter, etc.) or other means used to ensure that animals can control their thermoregulatory environment. Include a description of IACUC/OB approved exceptions, if applicable. [Guide, p. 43]

Temperatures are set below the species-specific thermoneutral zone for most rodent species especially to avoid heat stress in the animals and for the comfort of the animal care staff. Animals can control their thermoregulatory environment by huddling together, as group housing is the default housing arrangement for social species as mandated by the ARC (http://ora.research.ucla.edu/OARO/Pages/ARC-policies/social-housing.aspx), through the use of contact bedding (rats, mice, pigs, etc.) and other forms of ARC-mandated environmental enrichment (nesting material in mice and rats, nesting boxes for birds, nesting huts in mice, PVC tubes in rats, etc.; http://ora.research.ucla.edu/OARO/Pages/ARC-policies/enrichment.aspx). ARC-approved exceptions to group housing and enrichment policies can be found in Appendix 18.

2. Ventilation and Air Quality [Guide, pp. 45-47]

a. Describe the methods and frequencies of assessing, monitoring, and documenting the animal room ventilation rates and pressure gradients (with respect to adjacent areas).Note: If preferred, this information may be provided in a Table or additional Appendix.

Ventilation in the animal rooms is 100% non-recirculated course-filtered fresh air. The ventilation system is designed to provide a minimum of 10 air changes per hourto all animal rooms and a minimum of 6 ACH to procedure rooms. Differential air pressure is balanced for each room as positive to exclude (i.e.: clean cage wash and many transgenic mouse holding rooms) or as negative to retain possible pathogens spread or experimental hazards (i.e.: necropsy rooms, biohazard rooms, soiled cage wash). Upon request, Facilities Management adjusts the animal room ventilation rates and/or pressure gradients, otherwise they calibrate and adjust flows and pressure gradients at least annually as part of scheduled maintenance. Every 3 years, the DLAM Vivarium Maintenance Technician surveilles and reports room ventilation rates using an Air Flow Capture Hood in older facilities: CHS, Franz Hall, Warren Hall. Facility Management Engineering Department surveille and reports Room ventilation rates data using building animation system for newer vivarium buildings: MRL, Gonda, NRB, BSRB, CNSI and TLSB. Baulin-tubes™ are visually monitored within hazardous

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containment areas, while directional flow is manually checked by DLAM personnel in all other areas according to our Environmental Monitoring SOP. Any apparent air flow discrepancies or unusual odors in hallways are reported to Facility Management Service Engineering Staff for repair or adjustment to maintain animal room ventilation rates and/or pressure gradients within safe ranges

b. Describe ventilation aspects of any special primary enclosures using forced ventilation.

The majority of mice and a small percent of rats are housed in individually ventilated cages. The caging systems include HEPA-filtered supply air to each cage and either HEPA-filtered exhaust air (which in most rooms is vented into the building exhaust) or is directly vented into the building exhaust without being HEPA filtered. Most of the cages are operated as positive pressure, with cages in ABSL2 areas operated as negative.

c. If any supply air used in a room or primary enclosure is recycled, describe the percent and source of the air and how gaseous and particulate contaminants are removed.

All air in the animal holding rooms is 100% non-recycled air. Rehab Building is used by DLAM exclusively for equipment storage due to recirculated supply air between rooms.

3. Life Support Systems for Aquatic Species [Guide, pp. 84-87]

a. Provide a general description of institutional requirements for enclosures using water as the primary environmental medium for a species (e.g., aquatics).

Institutional requirements are generated through the ARC and are based on recommendations from The Guide. One of the ARC’s policies covers the housing of Xenopus and details housing; water; temperature; light cycle; feeding/nutrition; enrichment; transportation; record keeping requirements; and arrival and conditioning (Xenopus spp. Husbandry policy, http://ora.research.ucla.edu/RSAWA/ARC/Pages/ARC-policies/xenopus-husbandry.aspx). For species housed within DLAM-managed space, an SOP is in place for husbandry of lamprey and amphibians (Xenopus and Rana). For species including Zebrafish that are housed outside of DLAM-managed space, each investigator maintains his/her own SOP that details the husbandry, water quality parameters, quality assurance procedures, stocking densities and monitoring, that is approved by the ARC. All of these SOPs will be available for review at the time of the site visit, upon request.

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b. Provide a general description of overall system(s) design, housing densities, and water treatment, maintenance, and quality assurance that are used to ensure species appropriateness.Note: Facility-specific tank design and parameter monitoring frequencies should be summarized in Appendix 12 (Aquatic Systems Summary).

The most common system design at UCLA is a filtered, continuous, and recirculating water system, with exceptions such as housing for tadpoles, which are housed in static tanks. Facility-specific tank design is included under Appendix 12 – Part 1. Housing densities for aquatics follow the recommendations of the Guide, including, for example, one adult frog (Xenopus or Rana) per gallon, and 40 adult lampreys per 100 gallon tank, within the DLAM facilities and in study areas. Tank densities for all aquatics species in all areas are included in Appendix 13. Water treatment within DLAM includes carbon filtration/dechlorination. Records of DLAM equipment maintenance (filter changes, calibrations, etc.) are available for review as instructed in Appendix 12. Quality assurance is assessed by weekly water quality parameter testing in DLAM-maintained areas, and retention of records in the room for inspection by the ARC. A non-DLAM-managed zebrafish core features a continuous recirculating modular tank system, with water that is dechlorimated, filtered (including a biofilter) and UV-treated. Details on this system (including the water quality testing) and other aquatic systems maintained outside of DLAM can be found in Appendix 12 – Part 2 and corresponding study area SOPs.

4. Noise and Vibration [Guide, pp. 49-50]Describe facility design features and other methods used to control, reduce, or prevent excessive noise and vibration in the animal facility.

To control for noise and vibration, service areas are located away from the animal rooms wherever possible. Noisy species such as dogs and pigs are housed as far away as possible from rodents (e.g. most dogs and pigs are housed on a separate floor of the CHS building). Solid versus hollow core doors help in noise reduction. Noise-conscious work habits are employed, e.g. using plastic litter carts, trash and feed containers, and proper maintenance (oil, grease) of equipment and food carts are used. If repairs or construction is required within an animal facility, attempts are made to relocate animals away from the noise, vibration and activity associated with such work. Sound batts have been built into the wall of the animal rooms during vivarium construction. Also, during a recent seismic retrofit project in the CHS building, a Noise and Vibration Impact Study was performed by an outside contractor and provided information that was used to relocate animals that would have otherwise been affected by the construction.

B. Animal Housing (all terrestrial, flighted, and aquatic species)

1. Primary Enclosures Note: A description of primary enclosures used (e.g., cages (conventional, individually-ventilated cage systems (IVCS), etc.), pens, stalls, pastures, aviaries,

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tanks) should be included in Appendix 13.

a. Describe considerations, performance criteria and guiding documents (e.g. Guide, Ag Guide, ETS 123 and/or other applicable standards) used by the IACUC/OB to verify adequacy of space provided for all research animals, including traditional laboratory animal species, agricultural animals, aquatic species, and wildlife when reviewing biomedical, field and agricultural research studies.

The Guide, AWA regulations, and CA Fish and Wildlife regulations (for some permitted species such as bats) provide guidance to ensure that we provide adequate space for all our species used in research.

b. Describe space exceptions to the guiding documents (Guide, Ag Guide, ETS 123, and/or applicable standards), indicating the references, considerations and performance criteria used (e.g., by the IACUC/OB) to verify adequacy of space provided for all animal species covered by the program. [Guide, pp. 55-63]

We have no institution-wide or ongoing ARC exceptions to the Guide regarding space. However, there are protocol-specific exceptions that the ARC approves on a case-by-case basis with consideration of the scientific justification that an investigator provides in the protocol. Examples of this include allowing an extra adult mouse in a cage with a litter of pups to co-raise pups that would not otherwise thrive without this extra assistance or allowing pups to remain with the mom(s) for an extra 7 days, typically, again to help pups of a certain weak transgenic strain that would not thrive on their own if weaned at the standard age.

2. Environmental Enrichment, Social, and Behavioral Management [Guide, pp. 52-55; 63-65: Ag Guide, Chapter 4]

a. Environmental Enrichment

i. Describe the structural elements of the environment of primary enclosures that may enhance the well-being of animals housed (e.g., resting boards, privacy areas, shelves/perches, swings, hammocks).

Most rodents are housed on contact bedding, which allows expression of species-typical behaviors such as digging.

Some rodent cages are equipped with tunnels or huts within the cage. Gerbils have stainless steel huts. Guinea pigs have PVC tubes or huts for hiding. Most birds are housed in large cages that allow for flight and have multiple

perches, swings and nest boxes. Birds housed in smaller cages have perches. Pigeons have cut bricks for resting off the floor.

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All NHP cages have perches and some cages have tunnels attached. Chinchillas have upside down rat cages to create a shelf and PVC pipes for

hiding. Geckos in DLAM-managed areas have PVC tubes for hiding. Xenopus frogs in DLAM-managed areas have privacy areas (PVC tubes). Other enrichment in PI-maintained study areas (such as plastic hanging plants

for bats and multiple hanging toys for birds) are detailed in the PI’s SOP for each individual SA and approved by the ARC.

ii. Describe nonstructural provisions to encourage animals to exhibit species typical activity patterns (e.g., exercise, gnawing, access to pens, opportunity for exploration, control over environment, foraging, denning, burrowing, nesting materials, toys/manipulanda, browsing, grazing, rooting, climbing).

Mice have nesting material. Singly housed Rats have Nyla-bones or similar items (paper twists) for

gnawing. Rabbits have PVC pipes, plastic chains or balls and hay. Pigs have sanitizable toys such as Kong toys or plastic balls, as well as turf

brushes for rubbing and scratching. NHPs, rabbits and pigs have at least one species appropriate hanging toy

(plastic chain, rattle, mirror) and at least one species appropriate floor ‘push’ toy (ball, barbell, Kong, PVC tube, wood, etc.) in their cage at all times. These items are rotated weekly.

NHPs have a play cage for exercise; climbing, swinging, standing, walking/exercise time provided on a rotating schedule.

Rabbits have a play cage for exercise and species typical behaviors such as sprinting and standing up on their hind limbs– exercise time provided on a rotating schedule

NHP cages have forage boards – seeds, raisins and other small treat items are placed to encourage foraging behavior

Chinchillas are provided wheels on a rotating basis for exercise All USDA covered species are provided with a variety of food treats (fruits,

vegetables, seeds, cereal, etc.) on a rotating basis. Depending on the species, frequency given varies from 2-7 days a week. Some treats are placed in devices to encourage species typical behavior (forage boards, wire springs, challenger balls).

b. Social Environment [Guide, p. 64]

i. Describe institutional expectations or strategies for social housing of animals.

Social management, group-, or pair-housing is implemented for all social specieshoused within DLAM when individuals are observed to be compatible. Social housing is the default housing arrangement for social species as mandated by the

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ARC (http://ora.research.ucla.edu/OARO/Pages/ARC-policies/social-housing.aspx).

ii. Describe exceptions to these expectations (e.g., veterinary care, social incompatibility) and other typical justification approved by the IACUC/OB for housing animals individually.

There are some general exemptions to social housing: Temporary single housing of post-surgical animals Breeder male mice, or male mice from certain aggressive strains that would

otherwise fight Adult male rabbits d/t aggression Veterinary health reasons And some individual animal exemptions: Most NHPs are not socially housed, although there are some in the socialization

process. Several NHPs have permanent exemptions due to behavioral incompatibility.

There are also several rabbits that are not socially housed due to eye surgery or behavioral incompatibility.

There is currently one chinchilla not socially housed due to behavioral incompatibility.

At any given time we have several pigs and rabbits that are individually housed for lack of suitable partners.

Finally, scientific justification exemptions, e.g. due to special drug treatments or foods, interference with instrumentation such as cranial implants, or metabolic caging, etc. are listed in Appendix 18.

iii. Describe steps taken with isolated or individually housed animals to compensate for the absence of other animals (interaction with humans, environmental enrichment, etc.).

Single housing of social animals is limited to the minimum number and duration necessary. Singly housed animals are provided with visual, auditory, olfactory stimulation and sometimes increased human interaction, when appropriate and according to DLAMs enrichment program. Many single-housed rats, especially in our vivarium most closely associated with behavioral testing and research, are housed in open-topped wire bar lidded cages, which allow them to hear and smell other rats. Rabbits are housed in cages that allow them to see, hear and smell other rabbits. Depending on species, protected tactile contact with compatible conspecifics is offered whenever feasible. Isolated NHP are provided with increased human interaction. Isolated dogs receive daily positive human interaction.

Permanent exceptions to social housing and/or enrichment are documented for 84

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USDA covered species in their medical records. For rodents, reasons for single housing are noted on the cage card. Regardless of USDA-coverage, all animals are provided with environmental enrichment, unless withholding enrichment is described in the protocol and approved by the ARC. Specific details are noted in Appendix 18. DLAM SOPs outlining enrichment and behavioral and socialization procedures for each species, including documentation, are available for review at the time of the site visit, upon request.

c. Enrichment, Social and Behavioral Management Program Review [Guide, pp. 58, 69]Describe how enrichment programs and exceptions to social housing of social species are regularly reviewed to ensure that they are beneficial to animal well-being and consistent with the goals of animal use.

The committee and DLAM veterinarians review the ARC’s environmental enrichment policy (http://ora.research.ucla.edu/RSAWA/ARC/Pages/ARC-policies/enrichment.aspx) periodically. Housing exceptions, including requests for single housing of social species or requests to withhold standard enrichment items, are reviewed at the time of initial and de novo protocol review or when a relevant change is made to a previously approved activity.

The dedicated Environmental Enrichment Coordinators within DLAM, with representative members of the vet staff and animal care staff, meet monthly to review, assess, and update the enrichment program. In general, each species and their behavioral management and training program are periodically discussed in depth. In between formal meetings, the veterinary and animal care staff members discuss individual cases as needed.

Animals showing abnormal behavior are reported to the veterinarian, who examines the animal and treats or manages the case as needed. Negative behaviors that may be specific to enrichment/social housing include stereotypical behavior, alopecia, fighting and excessive aggression, or passivity to staff. When these signs are noted, the veterinarian considers behavioral as well as medical causes, and formulates an appropriate treatment plan. Laboratory members may also report abnormal signs to the veterinarian for evaluation.

The veterinarian also reviews temporary primate and dog exemptions at least every 30 days. For all other covered species, exemptions are communicated to the attending veterinarian for review at the time that the veterinary or animal care staff feels that an exemption is necessary, or on a monthly basis.

Animals that exhibit normal well-being and species-typical behavior, such as good appetite, appropriate behavior toward staff and conspecifics, appropriate behavior during study procedures, and appropriate study responses, are considered successful

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examples of the effectiveness of our enrichment program.

d. Procedural Habituation and Training of Animals [Guide, pp. 64-65] Describe how animals are habituated to routine husbandry or experimental procedures, when possible, to assist animals to better cope with their environment by reducing stress associated with novel procedures or people.

Animals arriving at UCLA are required to undergo an acclimatization period prior to being used for experimentation. This allows animals to habituate to the new environment and the routine husbandry procedures. For rodents, the acclimatization period is 72 hours; for covered species the acclimatization times is longer (up to 2 weeks for dogs and pigs, 31 days for NHPs).

Habituation and training are accomplished by the following methods: All appropriate personnel are trained in handling each animal species, and in

performing specific techniques outlined in the SOP or experimental protocol, so that routine husbandry and experimental procedures cause as little stress as possible. DLAM staff members are trained by their supervisors, and laboratory members are trained by DLAM’s training personnel.

Positive human interaction is accomplished by Animal Care Technicians, Veterinary Technicians, and in some cases the veterinarian and lab members.

Whenever possible, the same Animal Care and Veterinary Technicians care for each animal area, to help familiarize the animal and habituate it to procedures. In addition, husbandry procedures are generally not changed, so that the animal is easily able to become used to them.

Positive reinforcement training, including clicker training, is incorporated into the training program for primates and long-term dogs and some pigs, unless exempted per animal use protocol or veterinarian.

We have also attempted to minimize stress associated with post-procedural care in USDA-covered species. When possible, long-term injectable medications are used instead of daily injections, oral medications are given (in palatable form or in a treat) rather than injections of the same drug, and treats are given after protocol manipulations such as eye ointment administration.

e. Sheltered or Outdoor Housing [Guide, pp. 54-55]i. Describe the environment (e.g., barn, corral, pasture, field enclosure, flight

cage, pond, or island).

The only outdoor housing is a series of 7 outdoor enclosures on the 8th floor of the CHS vivarium used for housing swine. The runs are constructed of fiberglass sides, chain link doors, and poured epoxy floors.

ii. Describe methods used to protect animals from weather extremes, predators, and escape (windbreaks, shelters, shaded areas, areas with forced

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ventilation, heat radiating structures, access to conditioned spaces, etc.).

Weather extremes are unusual in West Los Angeles. Nevertheless, DLAM vivarium supervisors and veterinarian team monitor the LA weather forecast. Infrared heaters are provided when cold weather is predicted during winter months. Animals may be relocated indoors during periods of extreme weather. About 90% of the area of the outdoor runs are covered with fiberglass panels to provide shade and protection from wind. There is a cool water mister system in place for the pigs that is manually turned on when the ambient outside temperature exceeds 81° F. The entire run area is covered with chain link and protected by the vivarium security system. The open top of this area is under surveillance by a security video camera.

iii. Describe protective or escape mechanisms for submissive animals, how access to food and water is assured, provisions for enrichment, and efforts to group compatible animals.

Animals are typically grouped by compatibility in pairs or groups in either indoor (rabbits, chinchillas, pigs, dogs) or outdoor (pigs) enclosures. More than one lixit and feeder are made available, so that subordinate animals are able to eat and drink. Animals are weighed monthly at a minimum (if not specified more often as per ARC-approved experimental protocol), and significant weight losses or other abnormal signs are communicated to the veterinary staff. Animals are monitored daily for signs of inadequate body condition, illness or stress. Both the Animal Care and Veterinary technicians under the supervision of the Environmental Enrichment Coordinator attempt to find appropriate groupings, if initial groups or pairs appear incompatible.

f. Naturalistic Environments [Guide, p. 55]

i. Describe types of naturalistic environments (forests, islands) and how animals are monitored for animal well-being (e.g., overall health, protection from predation).

UCLA has no naturalistic environments.

ii. Describe how food, water, and shelter are provided.

N/A

iii. Describe how animals are captured.

N/A

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C. Animal Facility Management

1. Husbandry

a. Food [Guide, pp. 65-67]

i. List type and source of food stuffs.

The below list includes standard diets and those chosen by DLAM veterinary staff to treat or prevent certain conditions, such as fenbendazole diet to treat pinworm infestations in mice. Other experimental diets may be fed according to ARC-approved protocols.

Mice, rats - Purina Lab Diet 5001, Purina RMH 2000, Purina Lab Diet Irradiated 5053, Purina Lab Diet irradiated 5LJ5, Purina PicoVac 506, Envigo Rodent Diet 7013, Envigo Rodent Diet 8604, Envigo Irradiated Diet 7904, Lab Diet Certified Rodent Diet 5002 (for mice or rats in GLP studies), and Irradiated Envigo 2018 and 2018S Fenbendazole and Uniprim Diets.

Rabbits - 5P26 Pro-Lab Diet; Certified Rabbit Irradiated diets for immunosuppressed rabbits and for rabbits enrolled in GLP studies.

Pigs - ProLab 5P94. Dogs - Purina LabDiet for Dogs 5006. Geckos – Live crickets (dusted with a calcium supplement); dried fruit flies. Frogs (adults) – Frog Brittle from Nasco for Xenopus, also frog kibble and

fresh beef liver. Bullfrogs receive mealworms. Frogs (tadpoles) – tadpole diet (ground alfalfa powder, Tetra or Omega One). Chinchillas - Mazuri 5M01 (Purina). Non-human primates - Teklad 5038. Gerbils - Purina Lab Diet 5001. Hamsters - Purina Lab Diet Irradiated 5053. Pigeons - Mix manufactured By Leach Grain & Milling Co., Downie CA

90241. Guinea Pigs - Purina Lab diet 5025. Lamprey – are not fed while housed at UCLA as per ARC-approved protocol

1993-230. Chickens (as chicks) – Newco 15065 Lab Diet Chick Start and Grow (or

equivalent) Fish – zebrafish / Medaka: brine shrimp, Golden Pearl Larval Diet, dry flake

food, "baby food powder"; Tetra, Omega One, Zoo Med. Salamanders – live crickets (dusted with protein- and calcium-powder),

Petsmart. Toads – live crickets (dusted with protein- and calcium-powder), Petsmart. Axolotls – Rangen Soft Moist Axolotl pellets. Newts – frozen bloodworms, Petsmart. Birds (finches) – birdseed mix (Royal Feed, Leach Grain & Milling Co), bird

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health grit (Royal Feed), cuttlebone, whole grain bread, hard-boiled eggs, shredded lettuce.

Bats – fruit bats: Daily fresh fruits (varying composition of bananas, oranges, mangoes, grapes, etc., depending on the seasonal availability; horseshoe bats: mealworms dusted with multivitamins and minerals.

Enrichment food items (in DLAM-managed areas): fruits and vegetables from Ralph’s Grocery Store (reputable grocery chain with locations throughout Southern California); food treats from BioServ.

Other supplementary foods may be given by veterinary discretion to increase caloric intake, such as: Oxbow Critical Care for rabbits; Clear H2O DietGel Boost Recovery for mice/rats; canned commercial dog food for dogs; Ensure liquid dietary supplement for pigs.

ii. Describe feed storage facilities, noting temperature, relative humidity, and vermin control measures, and container (e.g., bag) handling practices, for each of the following:

vendors (if more than one source, describe each) centralized or bulk food storage facilities if applicable animal facility or vivarium feed storage rooms storage containers within animal holding rooms

VendorsNewco: Animal feed is purchased from Newco Distributors, an ISO 9001:2008, AIB Certified LabDiet distributor. Laboratory diets are stored in an environmentally monitored 22,000 sq. ft. cement building. The roof height is 27 feet. This warehouse is equipped with a thermo hygrometer. The warehouse is cooled by an industrial A/C unit. All lab products are secluded in a barrier curtain to ensure additional protection. All products are stored on pallets off the floor away from walls. Feed is monitored, tracked and rotated to assure freshness by date code. Feed is manufactured exclusively in the Purina Mills ISO 9001:2008 plant in Richmond, IN. No antibiotics, synthetic estrogen, or other such chemicals enter the facility. Only FDA and AAFCO approved feed additives for feed nutritional uses are permitted in the facility. Both Purina Mills and Newco Distributors, Inc. have certified pest control services for their facilities. Rodent control is accomplished with bait stations on the outside of the facility. Nontoxic glue boards are used in the interior of the facility. No pheromone traps for flying insects are used. Further insect control is conducted by a certified pest control service utilizing Pyrethrin - Piperonyl butoxide when necessary. Damaged or spilled product is removed and discarded immediately after found.

Envigo, Inc. Teklad diet & bedding storage Warehouse Standards &Procedures: Climate Control - The entire diet storage facility is fully climate-

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controlled. Temperature is controlled never to exceed 70oF. Relative humidity not to exceed 55% in the warmer months. Temperature and humidity are monitored and recorded daily, and records are available upon request. Vermin Control - Glue boards are located every 10 to 15 feet throughout each warehouse. Pheromone traps. Managers walk the entire perimeter of facilities daily. Additionally, an independent pest control vendor is contracted for each facility to supplement in-house program. They inspect warehouses and feed mill facility twice per month.Inspection of Incoming Materials - Pallets of product entering facilities are carefully inspected for signs of damage or vermin infestation. Routinely re-palletize incoming bedding material as an extra precautionary measure in checking for signs of vermin activity. Product is rotated and stored using a FIFO (first in, first out) inventory rotation system.

Nasco: Xenopus frog brittle food is manufactured exclusively for Nasco by PurinaMills. The vendor orders 4,000 lbs at a time. The bulk food arrives in waterproof,triple-lined bags. It is stored in 50 lb bags, on metal shelving, in the Biologywarehouse. Warehouse temperature varies from 60-80oF. The warehouse is made of poured concrete with mesh screen metal shelving. Pesticides are not used andinventory is rotated frequently.

BioServ: Bio-Serv is an ISO 9001:2008-compliant manufacturing company located in Frenchtown, NJ. Depending on the product, storage is either in a cool room (~65oF), refrigerated walk-in cooler (~40oF), freezer (~5oF), or in an ambient temperature warehouse (~75oF). All temperature-controlled areas are monitored for compliance to the temperature range. Employees clean all areas routinely. Outside pest control company services facility bi-weekly and uses only traps; no chemical sprays. Products are shipped to customers via UPS, FedEx, or Common-Carriers. Bio-Serv does not have its own delivery service.

Clear H2O: Clear H2O is a Maine-based life sciences company with an FDA approved HAACP facility (hazard analysis and critical control points) that is inspected by Siliker, NSF Cook & Thurber and also undergoes a third-party inspection. All of their products are tested and receive a certificate of analysis. Products are received from the manufacturer through the DLAM Pharmacy and stored there until dispensed / used.

Centralized/bulk food storages areasN/A

Foodstuffs for exotic species are purchased through DLAM’s central vendor (Newco) or from reputable commercial suppliers (such as Petco). Fresh fruits, vegetables and other foods (such as eggs) for these species are purchased from local grocery stores, washed and stored refrigerated as needed.

Animal Facilities

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Feed is delivered weekly and stored within each animal facility off the floor and 6 inches away from the walls. Room environment is maintained according to Guide standards and is monitored daily. In feed storage rooms where the temperature fluctuates from the permissible range (there is at least one location like this), food is stored for a maximum of 2 weeks and then replaced. Perishable fruit and vegetables are kept refrigerated. Product is stored and rotated using FIFO (first in first out) inventory rotation system. All feed storage locations and laboratories are included in the pest management program: vermin control is accomplished via exclusion barriers, immediate sanitation of any spilled product, daily observation for any signs of infestation, and use of sticky traps for insects.

Animal Rooms and RunsIn animal rooms and runs with DLAM-managed vivaria, for feed that arrives in large bags, each is placed (usually in its original bag) into large plastic bins with tight fitting lids off the floor and on dollies. A label with the type of feed is attached to the lid of the bin. The bags each have milling dates, which remain with the bag. For other types of feed, they are stored in secure, plastic containers with an expiration date or milling date of the food clearly visible. If the foodstuffs are any material that might be suitable for humans, the notice “not for human consumption” is included on or in the storage container.

iii. Describe special food preparation areas, such as feedmills and locations where special diets are formulated, if applicable. Include in the description sanitation and personnel safety practices (noting that respiratory protection is described in Section 2.I.A.2.b. ii. Standard Working Conditions and Baseline Precautions above).

CHS 8V-221, BRI X3-399 & X3-399C, and NRB X20K are used to prepare food used for environmental enrichment.

For 8V221, the main food enrichment room, the sanitation and food safety practices are as follows: Daily (excluding weekends and holidays): Empty trash (daily or as needed);

Wipe down sink and countertop (daily or after each use); Wash cutting boards and utensils after each use.

Weekly: Wash enrichment food containers; Check all food inventory; discard expired or spoiled items; Sanitize floors.

Monthly: Sanitize refrigerator/freezer; Sanitize horizontal and vertical surfaces. Other: Sanitize bins used to store non-perishable food treats between stock

replenishment Perishable food is purchased weekly to keep stock low and prevent spoiling. Food supply is checked M-F and old/spoiled items are discarded if necessary. Food items are taken from the enrichment room on a first in, first out basis or

according to nearest expiration date. Fruits and vegetables are washed (rinsed with water) prior to distribution to the

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animals Food treats with the exception of fresh fruits and vegetables are labeled with a

minimum of one of the following: milling date, expiration date or date of receipt.

Fruits and vegetables that have been cut are stored within the refrigerator in a food container or ziplock bag and labeled with the date placed in the container/ziplock. Contents are used or discarded within 1 week.

Room temp and humidity are checked and recorded daily Refrigerator and freezer temperatures are checked and recorded daily

The above items are documented on a room maintenance log.

For the BRI NHP area: DLAM maintains a small refrigerator for perishable food storage. When the

NHPs are on study, DLAM leaves the food treats for the lab personnel to distribute to the monkeys. A cleaning log is used to document cleaning tasks in this area as well.

DLAM also stocks and maintains the dry food treats Food containers are washed between stock replenishment. Food storage bins are sanitized monthly and logged on the back of the room status sheet.

Cutting boards and utensils are washed after each use.

For the NRB NHP area: The refrigerator belongs to the PI lab. Perishable food items are retrieved from

the 8V EE room by DLAM staff and stored in the lab’s refrigerator for short term (usually no more than 3 days worth of food treats are stored at a time). The lab members distribute the treats to the NHPs. The lab is responsible for checking and discarding the perishable food items as well as sanitizing the refrigerator. The lab keeps a monthly sanitation schedule log.

DLAM stocks and maintains the dry food treats. Food containers are washed between stock replenishment. Food storage bins are sanitized monthly and logged on the back of the room status sheet by DLAM staff.

iv. Describe how food is provided to various species (ad libitum, limited amounts, types of feeders).

Information below reflects standard practice. Variations may occur and would be reflected in ARC-approved protocols.

Mice, rats - ad lib in suspended feed hopper. Rabbits - fed 8 ounces per day in J-feeder (less if animal is <2 kg in body

weight). Pigs - fed an amount based on the body weight of the animal (approx. 1 pound

of food per 25 pounds of body weight), in a feed bowl on the enclosure floor. 92

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Dogs - fed an amount based on the body weight of the animal, in a feed bowl on the enclosure floor.

Geckos – limited amounts (2-3 crickets up, 3 times per week up to daily), given to geckos in their home cages.

Frogs (adults) - measured amount in tanks. Frogs (tadpoles) – one pinch, delivered to home tank. Chinchillas - ad lib in J-feeders. Non-human primates - fed an amount based on the body weight of the animal in

feeders. Gerbils - ad lib in hopper and on cage floor ad lib in hopper and on cage floor. Hamsters - ad lib in hopper and on cage floor. Pigeons - measured amount of bird seed in bird feeders, as fed by principle

investigator lab staff. Guinea Pigs - ad lib in J-feeders. Lamprey – not fed while housed at UCLA as per ARC-approved protocol 1993-

230. Chickens (as chicks) – ad lib in J-feeders Fish (zebrafish and Medaka) – hand-fed 2 -3 times per day, in the tanks. Fish (other species) – fed 2- 3 times per week, commercial fish food (flake

food), in home tanks. Salamanders – hand-fed crickets 3 times per week, in home enclosure. Toads – hand-fed 1-2 crickets per toad 3 times per week in home enclosure. Axolotls – fed 2 – 3 times per week, Rangen Soft Moist Axolotl pellets, 5 mm

pellets, given in home tank. Newts – hand-fed a measured amount of dried bloodworms three times per

week in home enclosure. Birds (finches) – ad lib birdseed in bird feeders, with supplements and treats as

specified in lab SOPs. Bats – daily replenishment of multiple-unit feeding stations (both species); food

may be withheld one day per week to prevent overfeeding.

Weights of covered species are monitored at least monthly (more often if indicated in experimental protocols) within DLAM-managed vivaria and the feeding regimen is adjusted as necessary. Ad lib diets are adjusted for food restricted protocols and dietary restrictions, or as per veterinary instructions.

Enrichment food items are provided in various forms that facilitate the expressionof species-typical behaviors.

v. Describe special food quality control procedures including procedures for rotating stock, monitoring milling dates, nutritional quality, bio load, chemical contaminants, etc.

Every pallet of product that enters the facility is thoroughly inspected for signs ofdamage or vermin infestation. Damaged, outdated or visibility contaminated

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product is not accepted into the facility. All animal food is stored and rotated using a FIFO system. Temperature and humidity are closely monitored and only enough feed is ordered to last approximately two (2) weeks in DLAM areas so that food is used quickly and close to its milling date. For mice and rats, much of the food is irradiated by the vendor or autoclaved before use. GLP studies require certified diets.

b. Drinking Water [Guide, pp. 67-68]

i. Describe the water source, treatment or purification process, and how it is provided to the animals (e.g., bowls, bottles with sipper tubes, automatic watering, troughs, ponds, streams).

Drinking water is obtained from the city of Los Angeles municipal water supply,which is potable and of excellent quality by all measurable health standards. On our campus we supply water to the animals by use of automated watering systems (AWS), water bottles with sipper tubes, or water pouches (Lab Products’ Hydropac®). A water bottle filler provides water for most rodent rooms. Additional treatment such as medicating or acidification is provided per approved protocols (e.g. acidified and reverse osmosis [RO] water for immunocompromised rodents).

Large animals housed in rack caging or runs, and not restricted by a research protocol or special condition, receive water from an AWS, which is equipped witha 5-micron water filter.

Rodents in various facilities may receive RO water from an automated system (SE Lab Group). Mice, rats, guinea pigs, hamsters, gerbils, chinchillas and rabbits are typically provided water bottles with sipper tubes. In the Radiation Oncology facility, all water bottles are autoclaved.

RO-filled Hydropac® water pouches or water bottles and holders are available to substitute for the AWS on rack caging in case of system failure or when a specific protocol or condition requires their use.

Bats are provided multiple wall-mounted dishes of water, changed daily, supplemented with multivitamins two to three times per week. Group-housed finches have cage-mounted water bottles with sipper tubes, several per cage. Pigeons have individual water bottles. Geckos have water dishes in their enclosures, large enough for submersion; these are changed daily.

ii. Describe methods of quality control, including monitoring for contaminants.

The AWS is checked daily to ensure proper operation, i.e., water pressure, free flowing lixits, and abnormal leakages when in use. Water bottles are washed atleast every two weeks and/or at cage change. Potable water testing is performed

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quarterly by the DLAM Clinical Diagnostic Laboratory staff. Water samples are collected from each vivarium facility on campus and are tested in house in the DLAM Laboratory for Total Coliform by the ColiTag™ method. Results are compiled into a report that is provided to the DLAM managers. Follow-up testing is performed if any results are positive (any coliforms detected).

iii. If automatic water delivery systems are used, describe how they are maintained and sanitized.

The DLAM automatic water systems (AWS) are recirculating systems and are treated by UV radiation and RO. The systems are serviced annually as part of a preventative maintenance contract with SE Lab. UV bulbs are changed quarterly. Cage racks are flushed weekly. AWS for non-rodent species are filtered via 5-micron filter and changed monthly. Water lines are tested daily and flushed weekly. Lixits are charged upon placement of animal in the enclosure to confirm unrestricted flow of water. Water testing is performed quarterly, as described above.

c. Bedding and Nesting Materials [Guide, pp. 68-69]

i. Describe type(s) and how used for various species.

Both direct and indirect bedding materials are used in the vivaria. All bedding types are absorbent, free of toxic chemicals or other injurious substances. Materials are determined by species. Other bedding or caging types (such as wire-bottom caging for mice / rats, which would preclude the use of contact bedding) is as stated in ARC-approved protocols.

Mice, rats - (Direct) Sani-chip, Diamond-Dri/Alpha-Dri, Bed-o-Cob, Carefresh. (Indirect; rare exceptions) Bed-OCobs, Poly Pads cage liners or Paperchips.

Rabbits - (Indirect) Paperchips. Pigs – most pigs on Aspen shavings (Direct) (required for ABSL2 work or for

piglets); some pigs housed with no bedding due to location (e.g. outside or some runs).

Dogs – no bedding. Geckos – paper toweling or Tech board substrate. Frogs (adults) – N/A (aquatics). Frogs (tadpoles) – N/A (aquatics). Chinchillas - (Direct and Indirect) Paperchip. Non-human primates - (Indirect) Paperchips. Gerbils - (Direct) Sani-Chips. Hamsters - (Direct) Sani-Chips. Pigeons - (Indirect) Sani-Chips. Guinea Pigs - (Direct) Sani-Chips/Aspen Shavings. Lamprey – N/A (aquatics).

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Chickens (as chicks) – Techboard w/ card/paper liner Fish – N/A (aquatics). Salamanders – EcoEarth® Compressed Coconut Fiber Reptile Substrate. Toads – N/A (aquatics). Axolotls – N/A (aquatics). Newts – N/A (aquatics). Birds (finches) - Corn-cob and corrugated cardboard on the floor of the

aviaries. Bats – no bedding.

(N/A = not applicable.)

ii. Describe bulk bedding storage facilities, if applicable, including vermin control measures.

Bedding is stored as described for food in section C.1.a.ii above. Also, one-ton bulk bedding bags are stored in a storage room away from the walls, on pallets, and are monitored weekly. For exotics, as applicable, bedding is stored in closed containers. Vermin control as above.

iii. Describe quality control procedures, including monitoring for contaminants.

Bedding materials are purchase from the same supplier listed for feed (Newco and Envigo-Teklad) and their quality control (QC) programs were described in section C.1.a.ii above. Both vendors test their products routinely for microbiological and chemical contaminants. Envigo’s quality control and assurance documents for bedding contaminants are available on-line at: http://www.harlan.com/products_and_services/research_models_and_services/bedding_and_enrichment_products/contact_bedding

d. Miscellaneous Animal Care and Use Equipment

i. Describe motorized vehicles and other equipment (e.g., trailers) used for transporting animals, noting the type and how the cargo compartment is environmentally controlled, if applicable.

Animals and equipment are transported in two designated stake bed trucks equipped with power lift-gates, two climate controlled vans and a climate controlled box truck with A/C and temperature monitor in the cargo compartment and a window for visual inspection of cargo. Transportation of animals between buildings is done in these vehicles.

ii. Describe other animal care related equipment used in the animal care program (specialized equipment for exercise or enrichment, high pressure

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sprayers, vacuum cleaners, tractors, trailers, spreaders, etc.).

HEPA-filtered vacuum cleaners are used in SPF rodent facilities. Metered pressure sprayers with the capacity to mix water and disinfectant are

used in cage wash areas, cart washing areas, and dog and pig housing locations. Ten-gallon capacity wet/dry vacuum cleaners are available Floor scrub machines are used to strip and wax floors Electric Tugger is used to aid in moving large equipment safely Robot is used to empty soiled cages, wash and refill with clean bedding (in

BSRB cage wash area only) Automated Bedding Dispensers (CHS XV, NRB, BSRB, TLSB) Vacuum bedding disposal system (BSRB)

e. Sanitation [Guide, pp. 69-73]

i. Bedding/Substrate Change

1) Describe frequency of contact and non-contact bedding change for each species and enclosure type (solid-bottom or suspended) or pen.

In addition to the scheduled changes, all cages are checked daily foracceptable sanitation. Unusually soiled or wet cages are changed whenfound.

(Please note, those species without bedding – the aquatics [Frogs; Lamprey; Fish; Toads; Axolotls and Newts]; and Bats – have been excluded from this list.)

Species Contact or Non-contact

Solid Bottom or Suspended

Frequency

Mouse (micro-isolator)

Contact Solid Bottom Weekly

Mouse (IVC) Contact Solid Bottom Every other weekRat (micro-isolator)

Contact Solid Bottom Once or Twice Weekly

Rat Non-contact Suspended Once or Twice Weekly

Rabbit Non-contact Suspended Twice WeeklyPig No bedding Runs (hosed) Twice DailyPig Contact Runs Once or Twice

DailyDog No bedding Runs (hosed) Twice DailyGecko Contact Solid bottom WeeklyChinchilla Non-contact Suspended WeeklyPrimate Non-contact Suspended Daily

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Gerbil Contact Solid Bottom WeeklyHamster Contact Solid Bottom WeeklyPigeon Non-contact Suspended Once WeeklyGuinea Pig Contact Solid Bottom Twice WeeklyChicken (chicks) Contact Solid Bottom Three times

WeeklySalamanders Contact Solid Bottom Monthly

(complete)Zebra Finches Non-contact Suspended Once WeeklyZebra Finches Contact Solid Bottom Once or Twice

Weekly

2) Describe any IACUC/OB approved exceptions to frequencies recommended in the Guide or applicable regulations and the criteria used to justify those exceptions.

Current exceptions include: Newborn litters. While investigators are encouraged to place expectant

mothers in clean cages, DLAM staff has instructions to delay cage changing for up to 3 days if newborn litters are discovered at the regular changing interval (multiple protocols).

Diabetic or otherwise polyuric animals. Assessed daily and changed as needed (various protocols).

Fourteen-day uninterrupted telemetric recordings in mice or rats in micro-isolator caging (Protocol 1999-028)

3) Note the location where soiled bedding is removed from the cages/enclosures and where clean bedding is placed into the cages/enclosures.

In the newer UCLA vivaria (e.g. BSRB, NRB, TSLB), the soiled side of the cage wash rooms is used for removal of soiled bedding into a dump station (or “bedding disposal unit”) whereas the clean side is used to dry wash cages, and to dispense clean bedding into them before they are sterilized by autoclaving. In the older vivaria (e.g. CHS) we have no separate clean and soiled sides. In these cases, soiled bedding is removed in the cage wash room and clean bedding is filled in a designated room outside of the cage wash room.

Chinchilla, finches, gerbil, guinea pig, NHP, pigeons, and rabbit cage pans are emptied into a bedding waste bin and fresh bedding is placed into the pans all within the animal room. Disposable rodent cages are used in hazardous containment areas and bedding is not removed. The entire soiled cage is disposed of as hazardous waste.

For ABSL2 swine pens, solid waste and absorbent bedding from ABSL pigs is

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carefully scooped to avoid generation of aerosols and disposed of as biohazardous waste. Disinfectant is applied and allowed sufficient contact time followed by a rinse with non-pressurized water. Clean absorbent bedding is replaced following disinfection.

ii. Cleaning and Disinfection of the Micro- and Macro-Environments Note: A description of the washing/sanitizing frequency, methods, and equipment used should be included in Appendix 14 (Cleaning and Disinfection of the Micro- and Macro-Environment) and Appendix 15 (Facilities and Equipment for Sanitizing Materials).

1) Describe any IACUC/OB approved exceptions to the Guide (or applicable regulations) recommended sanitation intervals.

None, other than those already listed above in C.1.e.i.2 under frequency of cagechanging.

2) Assessing the Effectiveness of Sanitation and Mechanical Washer Function

a) Describe how the effectiveness of sanitation procedures is monitored (e.g., water temperature monitoring, microbiological monitoring, visual inspections).

Water temperature monitoring in cage washers is done by visual observation of temperature gauges. Additionally, temperature sensitive tape, temperature strips, equipment digital read outs are checked and/or select washers have a validation programmed which stops the cycle if water in the tank does not reach 180 degrees F.

Temperature tape monitoring is completed at least once per day, for each washer, when the equipment is run.

Microbial cage washer surveillance testing is performed quarterly. Cages are also tested by this method in laboratories where they are hand washed for study area housing. Contact plates with DE-neutralizing agar are used to sample five interior surfaces of three cages from each cage washer. Plates are incubated at 37°C for 24 hours and bacterial colony-forming units (CFU) are counted. Results for each cage washer are compiled into reports that are provided to the facility managers. CFU counts of <20 are considered acceptable. Cage washer function is examined and repairs or changes in technique are initiated if cage washers do not meet the minimum standard. Follow-up testing is performed to verify cage washer function after corrections are made.

Spore testing using Biological Indicators is performed weekly for all DLAM autoclaves in operation.

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b) Describe preventive maintenance programs for mechanical washers.

Mechanical Cage washers are evaluated regularly by: checking and cleaning jets daily, checking and changing filters at scheduled intervals, running temperature strips with at least one load daily, draining washer tanks when needed, checking detergent daily and replacing when empty. All mechanical Cage Washers are included in a preventative maintenance service contract.

f. Conventional Waste Disposal [Guide, pp. 73-74]Describe the handling, storage, method and frequency of disposal, and final disposal location for each of the following:

i. Soiled bedding and refuse.

Soiled bedding and refuse are collected in heavy-duty plastic bags, which are placed into leak proof durable plastic containers (Rubbermaid®) with lids. These plastic bags are tied off and removed when filled to ⅔ capacity (or at the end of each day if not filled up), and transported to the refuse dumpsters. These dumpsters are dedicated for animal facilities’ refuse; they have coverlids and are located in the loading area just outside of each facility. A trash removal contractor collects and hauls the content away to commercial dumpsites on a daily basis. The BSRB vivarium has a solid bedding vacuum system which removes (nonbiohazardous) soiled bedding from the cage wash room and deposits it in a sealed container outside the facility. When the container is full, a licensed contractor removes the soiled bedding to a recycling center. The Gonda vivarium has a Garb-el (bedding grinder) unit. DLAM has contracted with a waste hauling vendor to have all non-biohazardous animal bedding in all vivaria to be recycled. For labs housing mice and rats in study areas, DLAM has arranged for them to exchange the soiled cages for clean ones with bedding at dedicated vivarium locations. This eliminates the need for the majority of labs to dispose of soiled bedding on their own.

ii. Animal carcasses.

Non-hazardous animal carcasses are removed from cages, put into a sealed bag, and placed in designated carcass refrigerators in each building pending necropsy or tissue harvest (if needed) for up to 72 hr. Carcasses are removed from these refrigerators as needed and moved to the central carcass cold room as medical-pathological waste, from which they are picked up weekly or more often if needed, by a commercial contractor. Lab staff are also able to deposit animal carcasses into dedicated vivarium refrigerators or the central carcass cold room for disposal.

g. Pest Control [Guide, p. 74]

i. Describe the program for monitoring and controlling pests (insects, rodents, predators, etc.). Include a description of:

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monitoring devices and the frequency with which devices are checked control agent(s) used and where applied, and who oversees the program, monitors devices, and/or applies the

agent(s).

Major emphasis for controlling vermin is focused on good sanitary practices, eliminating breeding and refuge sites, and maintaining facilities to prevent vermin entry. To that end, all animal holding and support rooms, including the corridors, are swept and mopped, or washed down at least daily. Animal care staff visually monitor animal holding and support areas for physical deficiencies, such as cracks on doors, floors, walls, or ceilings that could harbor pests or contribute to their survival and propagation. Any sign of pests is monitored for daily according to DLAM’s Vermin Control SOP and reported to Facilities Management “Trouble Call Desk”; a work order is created and sent to the pest control contractor. The contractor’s pest control technician schedules a visit to inspect and set traps when reports of pest sightings are received. A commercial contractor (Terminix) provides pest control services under a contract with UCLA’s EH&S office. This contractor maintains baited rodent stations on the exterior of buildings to control wild rodents. When a feral rodent is identified within a building, the exterminators are summoned to trap/capture the escaped animal. Humane traps may be deployed by the exterminator; when traps are deployed, the contractor inspect the traps daily.

ii. Describe the use of natural predators (e.g., barn cats) or guard animals (e.g., dogs, donkeys) used for pest and predator control, if applicable.

N/A

iii. Note how animal users are informed of pesticide use and how animal users may opt out of such use in specific areas.

No pesticides are used in the animal facility while animals are present.

h. Weekend and Holiday Animal Care [Guide, pp. 74-75]

i. Describe procedures for providing weekend and holiday care. Indicate who (regular animal care staff, students, part-time staff, etc.) provides and oversees care and what procedures are performed.

Each weekend, a team of animal technicians led by a Senior or a Principal Animal Technician, is assigned on a rotating basis provide animal care and husbandry for all DLAM animal holding facilities (also, currently one staff member is assigned to weekends full-time). For holiday work schedules, additional animal care technicians are assigned to change animal cages and additional support technicians are assigned to operate cage wash and autoclave facilities, as needed. Weekend and

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holiday assigned animal care staff provides animal health checks, monitors and provides feed and water for all species of animals. Excessively soiled or flooded rodent cages are spot changed. Large animal cage runs are washed down each day. All animals are checked for presence of adequate amounts of food and water and for any problems that may require reporting to the on-call veterinarian. Veterinary technicians also work on a rotating schedule and provide animal health checks and treatments, as needed. Veterinarians are on call on a rotating schedule as well and are available by telephone 24/7. The veterinary technician reports to the veterinarian by phone or pager following completion of rounds, or before, if the situation appears to be an emergency.

ii. Indicate qualifications of weekend/holiday staff if not regular staff.

All weekend/holiday staff are regular DLAM staff.

iii. Describe procedures for contacting responsible animal care and/or veterinary personnel in case of an emergency.

DLAM personnel’s phone and pager list, along with the DLAM emergency phone tree number, is posted in all animal facilities and on the DLAM website. The animal users, including DLAM staff, are instructed to call the emergency phone tree number to contact the on-call veterinarian for all animal related issues and Facility Manager for facility issues. The on-call veterinarian and Facility Manager can be reached at all times after hours and on weekends and holidays. The animal resource managers and supervisors are listed on DLAM emergency contact list at physical plant and campus police department for emergency contact regarding facility and or security issues. The division’s Executive Director is to be promptly notified of all major issues regarding physical plant or security breaches.

2. Population Management [Guide, pp. 75-77]

a. IdentificationDescribe animal identification methods for each species (e.g., microchips, cage/tank cards, collars, leg bands, tattoo, ear tags, brands).

All animal enclosures have identification cards, which contain the following basic information: Investigator name, contact name and number, animal species, and protocol number. Other information, such as gender, weight, age, date of birth, date of arrival, and vendor are usually noted as well.

Guinea pigs, chinchillas, rabbits, guinea pigs, and pigs have ear tags. Gerbils have ear punches. Hamsters are generally housed individually. If compatible and group-housed,

individuals are identified by non-toxic ink marks on their cheeks (no mark, left cheek, right cheek, both cheeks). No more than four (4) are group-housed at any

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one time. If marks fade, they are re-applied by the lab. Dogs are individually identified with tattoos or USDA tags. NHPs are individually identified with tattoos. All rat and mice cages have cage identification cards. In addition, rodents may be

further identified by ear tag, ear punch or notch, or tattooing of either the toes or tail.

Leg bands are used for birds (pigeons and finches). Frogs are group housed in tanks with cage identification cards; frogs are identified

via photographs when necessary. Nontoxic marker pen may be used for temporary identification of rats, guinea pigs,

hamsters and mice. Bats are not individually identified until they are entered into experimental studies,

at which time bats are identified with small dots of differently-colored nail polish.

b. Breeding, Genetics, and Nomenclature

i. Describe the program for advising investigators on the selection of animals based on genetic characteristics.

Veterinarians advise investigators on appropriate animal genetic characteristics during the protocol pre-review process or when new investigators join our institution. In DLAM managed breeding colony vivaria, DLAM staff arranges consultations with investigators to discuss colony goals/plans. During this consultation, breeding colony managers discuss special genetic characteristics of strains that may aid in the successful breeding of the line and address any special husbandry or handling peculiarities. Veterinarians may also be consulted at any time if breeding results are not as expected, or offspring yields decline.

ii. Describe the program for advising investigators on using standardized nomenclature to ensure proper reporting of the identification of the research animals with regard to both the strain and substrain or the genetic background of all animals used in a study.

The use of standardized nomenclature is encouraged but not strictly enforced. Investigators seeking guidance on proper nomenclature for identifying genetically modified strains are directed to information hosted on the Jackson Laboratory web site. In DLAM managed breeding colony barriers, full strain names in correct standard nomenclature are requested from the investigators when a new colony is set up and entered into the breeding colony logs. In PI-accessed vivaria, investigators occasionally use shorthand versions of strain/line nomenclatures. DLAM veterinarians are available to provide assistance to investigators for additional information.

iii. Describe genetic management techniques used to assess and maintain genetic variability and authenticity of breeding colonies, including

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recordkeeping practices (Guide, pp. 75-76).

In DLAM-managed breeding colony vivaria, DLAM staff collect a small ear or tail sample for genotyping. Researchers are responsible for maintaining genetic information and providing instructions to DLAM for continued breeding, new crosses, or culling. All genetic information provided to DLAM by the researcher is recorded on the breeding colony logs and sent to the researcher weekly. Researchers are encouraged to use vendor-sponsored programs to assess genetic authenticity such as Jax’ Mice for Life Program which includes a background genome scanning service, regular replacement breeders, and personalized colony management.

iv. For newly generated genotypes, describe how animals are monitored to detect phenotypes that may negatively impact health and well-being. Note that the methods used to report unexpected phenotypes to the IACUC/OB should be described in section 2.1.B.1.c.ii, “Unexpected Outcomes that Affect Animal Well-Being.”

Investigators must describe any known or expected phenotypes and their appropriate management in their ARC protocol. During the breeding colony consultation, any expected phenotypes and communicated to the breeding colony manager. In cases where unexpected phenotypes arise, DLAM breeding colony staff report them to the DLAM veterinarian and the investigator. Appropriate care of unique phenotypes is determined on a case by case basis, and the ARC protocol is amended to reflect new knowledge regarding their care.

III. Veterinary Care [Guide, pp. 105-132] Note: Complete each section, including, where applicable, procedures performed in farm settings, field studies, aquatic environments, etc.

A. Animal Procurement and Transportation [Guide, pp. 106-109; Ag Guide, pp. 8; 45; 50-57]

1. Animal Procurement Describe the method for evaluating the quality of animals supplied to the institution (from commercial vendors, other institutions, etc.).

There are two routes by which animals may arrive at UCLA, one is termed “procurement”, which would be defined as being purchased through a DLAM-approved vendor, and the second would be through “import,” which would be through importation or transfer of animals from another institution, facility or collaborating investigator. DLAM has in place SOPs to define these procedures, as indicated below.

From animals that are ordered, all are ordered through a central procurement office in 104

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DLAM and obtained only from approved vendors that have been previously qualified by DLAM veterinarians having appropriate health monitoring programs for the species involved (any exceptions to this are noted below by species). We capture these processes in DLAM SOPs for Animal Procurement and Vendor Surveillance as part of our preventive medicine program for USDA Covered Species. Briefly: Vendors are USDA licensed and are evaluated for the existence of AAALAC

accreditation. Vendor site visits are made on an as needed basis at the discretion of the veterinary

staff. The general health and condition of incoming animals are evaluated and documented. Vendor health monitoring reports and preventive medicine programs are reviewed. In the event of a disease outbreak at a vendor's facility, in-house animals from the

respective vendor may receive additional diagnostic screening.

Additional information by species: Chinchillas, gerbils, guinea pigs, hamsters, chicks and rabbits: Approved commercial

rodent, chick and rabbit vendors provide health surveillance information. Dogs & NHPs: Dogs are ordered from class “A” dealers only. NHPs come from a

USDA licensed dealer or USDA-registered research facility. All dogs and NHPs come with a summary of health records including treatments, vaccinations or other preventive interventions.

Pigs: Swine vendors provide DLAM with a written outline of their health maintenance and surveillance programs.

Rats and Mice: Approved commercial rodent vendors provide health surveillance information that is reviewed at least quarterly by a DLAM veterinarian. Mice and rats coming from institutions classified as –non-approved vendors (that is, imports) are evaluated case-by-case based on health history and the investigator’s needs to determine what facility they may enter into, whether a quarantine and testing period is required vs. rederivation,

Frogs: Frogs (Xenopus and Rana) are received from approved vendors. The Rana are purpose-bred for research only.

Birds (pigeons/finches): Zebra finches were originally purchased from a commercial bird vendor of acceptable health status. After the original purchase, finches have been maintained at UCLA as a closed colony. Pigeons were purchased from Double T farm or received from other University of California vivaria with clean health status. Pigeons are long lived and new birds are rarely purchased (last receipt, 2009). Birds of all species are received, transported within their shipping container to the facility where they will be isolated, quarantined and eventually housed.

Bats were imported to UCLA from two sources, one internationally from China (wild-caught) and one internationally from another institution (Israel). Both required permits from CDC, USDA and California Fish and Wildlife and were inspected upon receipt by DLAM veterinarians.

Zebrafish come from a variety of sources as imports into the Core (non-DLAM-managed). DLAM veterinarian and/or DLAM import coordinator review health monitoring reports from sending institutions before receiving of the animals.

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Lamprey are received as an import from a collaborator of the Principal Investigator. There is no approved vendor for this species;.

Geckos (tokay) are ordered from the only available vendor on the West Coast for these animals.

Geckos (fat-tailed), salamanders, toads, axolotls, newts, and fish (other spp.) are either ordered through DLAM or obtained from a reputable exotic animal dealer or a pet store as imports, with DLAM veterinary permission beforehand and examination upon receipt, including collection of any diagnostic samples as deemed warranted. These exotic species may be difficult to locate with approved vendors and detailed health reports, so outside commercial vendors may be appropriate.

2. Transportation of Animals Describe how animals are transported between outside sources and the institution and within the institution, including loading, unloading, level of biosecurity, immune status and specific pathogen status (consider all species, including aquatic and semi-aquatic species).

Animals are transported to UCLA via air and/or ground transportation by courier service. Several vendors have their own transport vehicles. Animals are typically ground transported in environmentally controlled vehicles. Food and water provisions are species specific and may vary depending on transportation and season. Animals are delivered to our facility by way of unloading directly from the truck to the facility dock. Shipping cartons are inspected and then placed on a flatbed cart for delivery to their designated quarantine room. Shipping cartons are opened within the animal housing room and animals are inspected upon transfer to individual housing. Animals (typically mice and rats) may be transported by personal vehicle; an inspection by DLAM personnel is required for approval, and a form is completed (Animal Transport Inspection Form). Animals must be contained in approved shipping containers (IATA-approved or home cages) and may not be transported in vehicle trunk, bed of a pick-up truck or on top of vehicle.

Within UCLA, disposable, opaque, closable containers may be used for transport a small number of mice or rats (such as transporting one mouse to an investigator’s laboratory for euthanasia). Containers must either be disposable (such as treated cardboard pagoda boxes) or sanitizable. In general, animals being transferred from standard holding rooms to areas where bio-hazardous/radioactive materials are utilized cannot be returned to standard animal rooms unless approved by DLAM Management. All animals are moved between locations without direct exposure to other species. Animals considered contaminated by environmental exposure are not reintroduced to the colony and may be isolated or eliminated from the colony following evaluation of risk/benefit between veterinary staff and study personnel. Environmental safety personnel and human health services will be consulted when indicated.

Additional information by species: Chinchillas, gerbils, guinea pigs, hamsters, and rabbits: Small animal carriers or rodent

cages are used to transport animals within the institution 106

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Dogs: K9 transport cages are used within the institution. NHPs: NHPs are occasionally transported to the UCLA imaging facility across the

street. The animals are anesthetized, placed in a specially-designed covered primate carrier, and transported via DLAM van with DLAM personnel (veterinarians and / or veterinary technicians) monitoring the animal at all times.

Pigs: Pigs are transported in the vendors’ trucks to the institution and a pig transport cage (stainless steel, solid walls) is used within the institution.

Rats and Mice: When rodent cages are transported between the vivarium and investigators’ labs, the water bottle is inverted and the microisolator cage is placed inside a dark, opaque plastic bag being careful to ensure an adequate supply of air to the animals. In some areas, a paper bag is used instead.

Frogs: For transport within the facility, frogs are placed into black rubberized containers with a loose fitting lid or a large beaker containing home water within the secondary black rubberized container.

Birds (pigeons/finches): Within the institution, individual finches are placed in small transport cages with a handle and a door on swivel, and covered with an opaque plastic bag. For more than one bird, they are placed inside a regular breeding cage, covered with an opaque plastic bag, and placed on a cart for transportation. The study area for the pigeons is adjacent to the bird room, and there is no public corridor, thus the birds are hand-carried rather than caged for transport.

Semi-aquatic and aquatic species (salamanders, toads, axolotls, newts, geckos): May be transported from one room to another for teaching purposes by having their entire enclosure placed on a cart and the cart wheeled carefully between rooms.

Bats: Bats are transported from the housing area on the roof of the Life Sciences Building down to the lab in a small animal carrier.

Areas outside of UCLA: Mice are occasionally transported between other local UCLA affiliated, AAALAC-accredited institutions and our campus, as described and approved in an investigator’s animal use protocol. As part of the import/export process, instructions on transport between institutions is provided to the collaborating institution.

B. Preventive Medicine

1. Animal Biosecurity [Guide, pp. 109-110]

a. Describe methods used to monitor for known or unknown infectious agents. Note that if sentinel animals are used, specific information regarding that program is to be provided below.

Animals are obtained primarily from approved vendors that have been qualified by DLAM veterinarians having appropriate testing and/or vaccination programs for the species involved. Prior to shipment of canine and nonhuman primates, health records are requested and reviewed for acceptability by a DLAM veterinarian. Animals, regardless of species, arriving without authorization to ship either are returned to the vendor, isolated pending evaluation, or may be euthanatized upon receipt.

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For large animals, newly arrived animals are segregated from the resident animals until the end of the quarantine/stabilization period, and are cared for after resident animals. Physical exam, blood/fecal testing and vaccination appropriate to the species and protocol are carried out during quarantine. Animals are assessed daily by DLAM personnel and abnormalities are reported to the veterinarian, who performs appropriate examination and testing, including testing for infectious agents if they are a likely differential diagnoses. Potential tests would include culture, cytology, hematology, serum chemistry and PCR.

For rodents (mice and rats), a rodent sentinel program is maintained by DLAM according to the DLAM SOP Rodent Sentinel Program. Briefly, serological testing, parasitology, and when indicated from gross necropsy, histological examination of tissues, are performed on sentinel rodents from each room quarterly. Sentinel mice and rats are purchased by DLAM and are placed in all long-term, rodent rooms. When cages are changed, soiled bedding from colony animals is placed into the sentinel animal cages. Animals are necropsied and a basic virus panel is done at UCLA and PCR (e.g. for fur mites and pinworms) are submitted for testing at RADIL.

For uncommon species, DLAM veterinarians tailor monitoring programs based on risk assessment and current veterinary practices.

b. Describe methods used to control, contain, or eliminate infectious agents.

The major objectives of infectious disease monitoring are to first and foremost prevent disease entry, and when infectious disease does enter, to detect it expediently, contain it immediately, and eliminate it if possible and desired.

In general, to minimize disease entry we control for pests and vermin that could introduce or spread disease. DLAM management are responsible for assuring that pesticides or rodenticides are only utilized in approved areas by supervising the application of these agents within the animal facility. Quality laboratory animal feed is used and treated to avoid the introduction of potential pathogens (e.g. irradiated feed is ordered for our rodents). Perishable fruits, vegetables, and other dietary supplements and enrichment food items are ordered, received, stored, and used in accordance with instructions of DLAM Veterinarian. Clean, fresh potable water from the City of Los Angeles water supply is provided for all species. The quality of the water meets or exceeds the National Primary Drinking Water Standards established by the EPA and enforced by TNRCC.

At least once a year, an independent chemical analysis of vivarium water quality is conducted, and reviewed for compliance with the national standards. To further assure water quality, water samples are submitted for microbiological testing quarterly.

Animals that may be at higher risk for infection (for example, very young, 108

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unvaccinated, immunosuppressed animals) are kept isolated from the general population.

An animal care technician observes animals daily after arrival; abnormalities are reported to veterinarian staff. If a potentially contagious disease is suspected, the animal is euthanized or isolated from other animals until the disease has been successfully identified, treated and the animal is deemed to be noncontagious. In these cases, the housing room is placed under quarantine to reduce exposure and possible disease spread to the general animal facility population. A veterinarian notifies affected research personnel immediately and provides necessary training. Appropriate isolation equipment (gowns, shoe covers, etc.) is provided immediately outside the quarantined housing room. Depending on the infectious agent, additional testing may be instituted to determine the extent of the problem and a treatment or eradication plan developed and implemented after discussion with the affected researcher(s).

2. Quarantine and Stabilization [Guide, pp. 110-111]

a. Describe the initial animal evaluation procedures for each species.

Chinchillas, dogs, gerbils, guinea pigs, hamsters, pigs, and rabbits: receipt, initial evaluation and assignment by DLAM animal care staff. A veterinarian is called only if problems are noted. An animal health technician observes the animal within 24 hours of arrival and notifies the veterinarian of any problem.

Frogs (DLAM-managed): All frog species are visually inspected by DLAM animal staff as the animals are transferred from their transport container to their housing tank, and daily thereafter

Non-Human Primates: To be accepted for housing at UCLA, all NHPs must be accompanied by APHIS form 7020 (Acquisition, Disposition and Transport of Animals), Health Certificate signed by a licensed veterinarian, and TB test history. In addition, NHP’s coming from outside California must be accompanied by a permit from the California Department of Public Health and by APHIS form 7001 (Interstate and International Health Certificate). Nonhuman primates are allowed to acclimate to their new surroundings for at least 24 hours before beginning quarantine procedures, as described below.

Rats and Mice: Once the shipping crates are opened by the receiving technician, a veterinarian is notified of any animals found sick, injured or dead and may then decide whether or not to take the animals to be necropsied and contact the sender. Both the animal resource supervisor for the destination area and the rodent procurement office are notified of any discrepancy between the animals received versus the order specifications and of any sick, distressed, injured or dead animals. The sender/vendor and the investigator are notified as soon as feasible. Once mice or rats have been moved into their designated areas, they are examined on a daily basis, and any abnormalities are brought to the attention of a veterinarian via the web based REACTOR program.

Birds: All birds colonies (pigeons and finches) have been closed colonies at UCLA 109

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for many years; however, the procedure for new birds would be to establish an initial visual examination by a DLAM technician or a lab member at the time they are transferred from their transport box to an acclimation / quarantine cage. Chicks would also have an initial visual exam at unpacking.

Exotic species (geckos, fish, salamanders, toads, axolotls, newts), if not ordered through a DLAM-approved vendor, may require a veterinary examination within 24 hours of arrival at UCLA; the evaluation process for these species would be worked out between the researcher, DLAM and the ARC on a case-by-case basis.

b. Describe quarantine facilities and procedures for each species. For each species, indicate whether these practices are used for purpose-bred animals, random-source animals, or both.

The majority of animals acquired by UCLA for research purposes are purpose-bred animals. Some of the minor species (such as geckos, Xenopus, chinchillas, etc.) are not purpose-bred for research, but they are not random-source animals. The same practices are used for both types of animals. We have SOP 0204 Receiving and Quarantine/Acclimation of USDA Covered Species that describes: prior to procurement requests, delivery and minimum quarantine/acclimation periods for chinchillas, gerbils, hamster, rabbits, GP, dog, swine and NHPs:Additional Information by species: Amphibians: Amphibians are placed directly into tanks based on vendor and day of

receipt and are not mixed with resident animals. Chinchillas: Newly arrived chinchillas are placed within the same room as the

existing colony, but never in the same cage as a member of the existing colony. Based on history and clinical signs at the time of animal arrival, the veterinarian may request that new arrivals be treated with a fungicidal dust bath before animals become available for research use.

Dogs: Dogs are acclimated separately from the main colony for a minimum of 5 days prior to experimental manipulation as follows:

o A physical examination is performed within 5 days of arrival including the lab work if needed ( fecal parasitology, hematology and serum chemistry)

o Long-term dogs are tested for heartworm per veterinary discretion and are vaccinated when appropriate.

Gerbils: Gerbils are purchased from an SPF vendor. Newly arrived gerbils are placed within the same room as the existing colony, but are separated by cage based on the date of receipt.

Hamsters: Hamsters are purchased from an SPF vendor. They are singly housed at arrival and not individually identified – other than by cage card. Newly arrived hamsters are placed within the same room as the existing colony, but are separated by cage based on the date of receipt. Offspring may later be group-housed (up to 4 per cage) and be identified with non-toxic ink on their cheeks.

Guinea pigs: Guinea pigs are purchased from an SPF vendor and all health testing is viewed on line and evaluated by a veterinarian prior to shipping. Newly arrived

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guinea pigs are placed within the same room as the existing colony, but are separated by cage based on the date of receipt.

Non-Human Primates: Quarantine procedures conform to state and federal regulations set forth by the California State Department of Health Services, Centers for Disease Control, and the Animal Welfare Regulations (CFR 9, 1990). Animals are kept in quarantine for a minimum of 31 days (60 days for animals out of state) to comply with California State requirements. A longer quarantine is sometimes necessary to accommodate treatments and the requisite interval between TB tests (30 days apart). NHP are allowed to acclimate to their new surroundings for at least 24 hours before beginning quarantine procedures. If the NHP was TB tested within the preceding 30 days, this may be considered the first quarantine TB test. Otherwise, a TB test is administered after the 24-hour stabilization period, and the date of this TB test is considered the first day of quarantine during the initial physical exam. NHPs are anesthetized and given a thorough physical exam by a veterinarian. A qualified veterinary technician observes the animals until fully recovered from anesthesia. Any abnormality is reported to the veterinarian immediately. Diagnostic procedures, tattooing and weight determinations may be carried out by DLAM staff. The results of all tests and examinations are entered in the individual animal record. Diagnostic procedures include: TB testing and interpretation, hematology, serum chemistry, fecal parasitology, and may include rectal culture for species of Salmonella, Shigella, and Campylobacter. NHP’s may be released from quarantine when they exhibit no apparent abnormalities on physical exam, at least two consecutive negative TB tests, blood parameters within reference range, at least two consecutive negative fecal exams and rectal cultures, and a written authorization issued by the California Department of Health Services (required only for NHPs coming from out of state).

Pigs: All newly arrived pigs are often kept in a separate enclosure from the existing colony. During acclimation, pigs receive a physical assessment by a veterinarian or a qualified technician within 5 days of arrival. A fecal exam for parasites and occult blood may be performed. Iron/ivermectin injections are given when needed

Rabbits: Rabbits are generally purchased from one SPF vendor. Newly-arrived rabbits are placed within the same room as the existing colony, although in separate cages. Animals are observed for signs of wellbeing and adequate acclimation to new food. Rabbits received from other vendors as required by investigators’ research needs are isolated in separate rooms. Rats and Mice: Rats and mice received from approved vendors and arriving in

intact shipping containers do not need to go through quarantine. They are unpacked and placed in microisolator cages according to our Rodent Receiving SOP. All rodents obtained or transferred from other than approved commercial vendors, regardless of written health assurances, must undergo a minimum quarantine period (2-6 weeks)during which they will be screened and may be treated for a variety of common pathogens. This mandatory isolation period is required regardless of any animal health screening information that may be provided by the transferring institution.

Lampreys are quarantined within the same room as existing individuals, but in a

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new tank. Geckos (both tokay and fat-tailed) – for both species, new individuals would be

quarantined within the same room as other geckos but in new enclosures. Chicks – in the same rooms as previous individuals but in separate enclosures. Zebrafish – a separate quarantine room is maintained for the Core, with set

procedures for introduction of the eggs / embryos into the Core tanks. For other Zebrafish study areas, similar separate tanks and procedures are in place.

Fish (other spp.), Salamanders, Toads, Axolotls, Newts – those species that would be eventually group-housed would be kept separated from in-house individuals for at least 5 days. Testing of feces or other samples may be required by a DLAM veterinarian to determine health status / zoonotic potential for these new exotic species.

Birds (finches) – Colonies have been closed for some time, but any incoming birds would be kept separate in quarantine cages for 5 – 7 days. Fecal samples may be required to be submitted by veterinary staff for Chlamydia or other pathogen testing during this time period.

Bats – New bats are kept separated from the main colony. A veterinary or veterinary technician exam is conducted. Fecal or other samples are collected for analysis as health condition warrants. Visible external parasites (such as sarcoptic mites, if present) are removed manually by the PI. Bats are treated with a drop of puppy-strength Revolution® (selamectin) at the nape of the neck. All bats are housed within the investigator’s study area.

c. Describe the required/recommended stabilization period for each species.

Mice, rats – 72 hours (no acclimation required for non-survival procedures) Rabbits – 5 to 7 days Pigs – 2 weeks Dogs – 2 weeks All reptiles and amphibians – 72 hours Chinchillas – 5-7 days NHPs - minimum 31 consecutive days Gerbils – 5-7 days Hamsters – 5 -7 days Pigeons – 72 hours Guinea Pigs – 5-7 days Lamprey – recommend 5 days (non-survival tissue collection) Chickens (as chicks) – unless specified / requested in the protocol, at least 72 hours

acclimation recommended. Fish (zebrafish) – 72 hours. Fish (other spp.) – 72 hours. Birds (finches) – at least 72 hours before use. Bats – at least a 6-month separation from main colony (California and CDC

requirements).The stabilization times listed above permit adequate periods for physiologic,

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psychological and nutritional stabilization for most animals. If animals do not appear to have adjusted to their surroundings at the end of the routine stabilization period, noted for instance as a failure to begin eating, they would be brought to the attention of a DLAM veterinarian as a health case

3. Separation by Health Status and Species [Guide, pp. 111-112]

a. Describe the program for the separation of animals by species, source, and health status. If the animals in different status are not maintained separately, describe circumstances in which mixing occurs and explain the rationale for mixing.

The vast majority of the vivarium locations maintain separation of animals by species.

As noted above by species, animals may be separated by source until the quarantine and acclimation period is complete. All animals that may become ill during quarantine or conditioning may be replaced by the vendor, unless the condition is easily correctable. Vendors often do not replace sick mice or rats after they have been received in good health. Ill animals are typically evaluated by the staff veterinarian and placed under appropriate treatment. If treatment is not desirable or possible, then the ill animal is euthanized and a necropsy is performed if the illness is not clinically apparent

For rodents, animals are segregated by health status according to DLAMs rodent room classification system and outlined according to our Rodent Room Classification policy. Briefly, rodents are classified and segregated at the room level according to 3 main health status criteria/exclusion lists: barrier level exclusion, conventional level exclusion, and pathogen suspect/positive.

b. Describe situations where multiple species may be housed in the same room, area, or enclosure.

Occasionally, two species (mice and rats) may be housed in the same room, e.g. within a biohazard containment area, or for scientific reasons. DLAM training mice and rats are routinely housed together in CHS. The rationale for this is ready accessibility to training animals in the vicinity of the training room or the investigators lab. Whenever they share a room, however, rats and mice are maintained in microisolator cages, which are opened only under a Class II biosafety cabinet or laminar flow work change station and generally at least one species is in a ventilated rack. For other exotic species in study areas, multiple species may be housed in the same room in separate enclosures and micro-environments. In no situation are multiple species housed within the same enclosure.

c. Describe isolation procedures and related facilities for animals.

Animals showing clinical signs of illness or abnormal results from diagnostic 113

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procedures are evaluated by the veterinary staff. These animals may be observed, treated, isolated, or euthanized.

Dogs, primates, rabbits or swine showing signs of illness with a suspected contagious disease are separated from the rest of the group by placing them either in a separate room, or in a cage that negates contact with other animals, depending on the transmissibility of the disease.

Chinchillas, gerbils, guinea pigs, finches, Zebrafish, frogs, bats and hamsters with a suspected contagious disease are placed on a separate rack, in a cage or tank that negates contact with other animals, or are euthanized, depending on the transmission of the disease. Exotics may or may not be separated, depending on the veterinarian’s judgment as to the stress of isolation vs. the further risk of transmission to an enclosure-mate. A chick found with a suspected contagious disease, due to the short-term nature of the study and to the zoonotic concern of bird flu, would be euthanized and tested as a sentinel animal. Pigeons are individually housed as standard practice.

If an ill mouse or rat is currently group-housed with other mice or rats, the entire cage typically receives the prescribed treatment. The PI is notified of the illness, and asked if they wish treatment to be started by DLAM staff, or if the animal should be euthanized. If the PI believes the treatment may compromise the research, or the veterinarian determines that separation of the ill animal will improve its clinical outcome, the sick mouse or rat may be separated into its own cage for treatment.

C. Clinical Care and Management [Guide, pp. 112-115]

1. Surveillance, Diagnosis, Treatment and Control of Disease [Guide, pp. 112-113]

a. Describe the procedure(s) for daily observation of animals for illness or abnormal behavior, including: the observers’ training for this responsibility method(s) for reporting observations (written or verbal) method(s) for ensuring that reported cases are appropriately managed in a

timely manner.

The Procedure for Daily Observation: Every day all animals are observed daily by animal care technicians, and/or veterinary technicians during their routine rounds, or trained research staff. Daily health observations are made early in the regular workday by animal husbandry personnel. Investigative personnel also assume a role in observing and reporting the health and wellbeing of animals both in DLAM-managed areas and in study areas. Abnormal observations are reported to the veterinary staff daily. Direct and frequent communication between animal husbandry personnel, investigative personnel, and veterinary staff is considered imperative to assure accurate reporting and treatment of problems observed concerning animal health, behavior, and well-being. To help ensure the accuracy

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and consistency of health case reporting in study areas by laboratory staff, a DLAM veterinary technician performs weekly health checks on animals in these areas.

Their Training: All assigned technicians have been trained on the DLAM SOP Animal Health Check and are qualified to recognize abnormalities in the appearance of animals. Refresher training is provided at DLAM All Staff meetings each year. For investigator maintained animals, all research personnel are trained by the Primary Investigator (PI) to recognize sick or injured animals and to report injuries or illness to the PI and to DLAM vet services. In addition, DLAM provides an annual or semi-annual training class on recognizing and reporting sick or injured animals, to research staff. Weekly health check visits by the veterinary technician also include follow-up training and ongoing continuing education for laboratory staff in charge of animal care.

Method of Reporting for Rodents: the animal care technicians place a Post-it note on the cage and complete a written animal health report and submit to senior animal care staff. Senior animal care staff, e.g. Lead, Principal Animal Technician (PAT) or Supervisor, or veterinary technician enter the following information in their hand-held device or desktop computer: date, PI, contact, species, location and animals’ condition. A case is then created in the web-based program REACTOR where an email is generated and submitted to the PI and designees as to a recommended treatment. The PI can then reply and continue a dialogue with DLAM veterinarians, who can also be accessed by animal health technicians while performing their daily rounds. Investigators are contacted for cases that require immediate attention. A phone call may be followed by an email for documentation. Upon severity of the case a timeline of action is provided to the research team. If a PI does not reply within the time frame designated, the animal could be euthanized or treatment will be initiated. This system is also used for animals that are sick or injured in study areas as well, as reported by PI staff or found by the veterinary technician on the weekly visits.

Method of Reporting for USDA regulated species, aquatics, reptiles and birds: The animal care tech or AHT observe animals daily, with special attention to feed intake, fecal output, and behavior. When deviation from normal are observed, cases are reported to veterinary staff for further assessment. Veterinary Staff assess animals, then reports findings to the veterinarian(s) and describe the condition in the animal’s health record, if applicable (refer to SOP #0101 – Medical Records for USDA Covered Species). Veterinarian(s) assess the health case, contact the investigator if possible and decide on an action plan. Veterinarian’s action plan is executed by veterinary staff and/or investigators. All the events, assessments, and progress for non-protocol related issues are recorded in the animal’s health record.

Responsibilities of the research staff: OARO Policy ‘Notification of Investigators with Sick or Injured Animals’ (http://ora.research.ucla.edu/RSAWA/ARC/Pages/ARC-policies/veterinarian-

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notification.aspx) delineates the responsibilities and obligations of the Division of Laboratory Animal Medicine (DLAM) and Investigators concerning sick or injured animals. All principal investigators are required to report instances of sick or injured animals, including instances of post-operative complications, to a DLAM veterinarian or animal health technician immediately. This applies to animals housed in investigator maintained study areas, as well as DLAM facilities. It is not necessary to report instances of sick or injured animals if they have been euthanized according to the criteria for premature euthanasia listed in the associated Animal Research Committee (ARC)-approved protocol. Investigators may not initiate treatment of a sick or injured animal unless the treatment has been specifically described for an expected complication in an approved protocol or has been authorized by DLAM veterinary staff. The PI's lab is responsible for carrying out all treatments as prescribed by the veterinarian unless alternate arrangements for administration of treatment are made with DLAM. Animals not treated as prescribed may be euthanized at the discretion of the veterinarian.

b. Describe methods of communication between the animal care staff and veterinary staff and the researcher(s) regarding ill animals.

Animals found showing signs of injury, illness, behavioral issues or other abnormalities are reported to DLAM veterinary staff via a written animal health report or electronically via the REACTOR program. Urgent health problems are also reported to veterinary staff by phone (use of pager or DLAM phone tree will facilitate this communication). For mice and rats, communication between veterinary staff and researchers is primarily via REACTOR, or via phone for cases that require immediate attention.

c. Describe the preventive medicine and health management/monitoring programs (e.g., physical examination, TB testing, vaccination, hoof/nail trimming, teeth cleaning/floating, vendor surveillance, use of sentinel animals) for each species.

DLAM maintains a health surveillance program in which the health of animals from vendors and established colony animals is evaluated routinely. Surveillance diagnostics includes, but is not limited to serology, internal and external parasite evaluations, bacterial and viral culture, gross necropsy and histopathology. Other diagnostics such serum chemistries, hematology, and fecals are performed as determined by the veterinary staff and incorporated into the preventative health program as necessary.

Rodents. All rodents (mice and rats), including breeding colonies are housed in rooms monitored by a campus-wide Sentinel Animal Program. Swiss Webster or CD-1 mice and Sprague Dawley rats are assigned to groups of up to 70 rodent cages. Soiled bedding is collected from each cage within assigned groups at each bedding change and used for the sentinel cage. Mouse and Rat Sentinel animals are tested quarterly. The following tests are performed on one Sentinel animal per cage:

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o Gross necropsy with blood collection for serologyo Parasitology – performed on all mouse sentinels every quarter

A perianal cellophane tape specimen is examined for pinworm ova. Direct Ceco-colon content exam – for adult endoparasites. A cellophane tape specimen from the inguinal and nape of neck

areas is examined for ectoparasites.o Serologyo PCR: For “Higher Level Barriers” fecal material is collected for

Helicobacter PCR.o Histopathology – specimens are collected on grossly “abnormal” tissues

only. Tissues are sent to CHS 1st Floor Translational Pathology Core Laboratory (TPCL), or in-house for slide preparation and the slides are read by a veterinary pathologist.

o Bacteriology – specimens are collected only from suspect lesions and are sent to a veterinary reference laboratory (IDEXX) for culture and identification.

Rodents continued: Follow-up testing of individual cages may be initiated in rooms that have positive serology results with the exception of parvoviruses. Room-wide treatment is initiated in rooms that have positive parasitology results (for example, pinworms), followed by post-treatment retesting. Room SOP/Health Status signs are posted on all rodent rooms doors. Color/alphanumeric codes are used to indicate the health status of each room. Upon completion of all tests, results are compiled and a Sentinel Animal Report for each room is prepared. Based on the recommendation of the veterinarian, animals (including mice and rats) showing evidence of infection (e.g., abscesses or ocular discharge) may have samples collected from them and submitted to IDEXX for culture. Additionally, the veterinarian may request that any animal be submitted for a full necropsy exam at the time of euthanasia or when found dead to identify any trends in genetically modified animals or possible infections amongst a given population of animals.

Rabbits: Rabbits are weighed at receiving and then monthly and any significant weight loss is reported to the veterinarian. Rabbits are received primarily from an SPF vendor. Animals obtained from a non-approved vendor will be placed in quarantine and additional testing and prophylactic treatment received.

Pigs: When possible, prior to ordering, swine’s colony health status is checked by DLAM veterinarian, then, and based on standard veterinary practices and study needs, a tailored preventive program is designed for additional diagnostics tests and preventive treatments such as vaccinations and antiparasitics. Pigs are group examined and weighed at receiving, then weight is taken at least monthly, more often when pigs are on study protocols.. Animals may be checked for occult blood in feces as well as parasites and treated prophylactically with antibiotics and iron during the acclimation period.

Dogs: Prior to ordering, dog’s health records are checked by a DLAM veterinarian, then, and based on standard veterinary practices and study needs, a tailored preventive medicine program is designed for additional diagnostics test and

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preventive treatment for vaccinations and antiparasitics. Geckos: Tokay geckos are ordered from a DLAM approved vendor. Although only

one vendor exists for these animals on the West Coast, UCLA history with them has been good and animals received through them have been historically healthy. All receive an initial examination at receipt. No sentinel animals are used. If any wound be found dead during housing, they would be submitted for a full necropsy / testing as a sentinel animal for the population. Fat-tailed geckos are either ordered through an approved vendor or obtained from a reputable exotic animal vendor or pet shop, with DLAM veterinary approval and examination at arrival. Sentinel animals are not used. Diagnostic samples may be collected as needed from individuals.

Frogs (both Xenopus and Rana, DLAM-managed and study areas): All are ordered through DLAM-approved vendors. Sentinel animals are not used, but euthanized or found dead animals may be submitted for complete necropsy and sample testing at veterinary discretion. No preventative medicine practices are in place other than quarantine and isolation practices for sick or injured animals.

Chinchillas: Depending in the health status of the provider’s colony, chinchillas may receive a physical examination and are weighed upon arrival. At veterinary discretion, upon receipt, a small sample of animals may be evaluated (serology, gross necropsy, and histopathology) to determine current health status. Dust baths are provided to aid in health maintenance and grooming and in the treatment for ringworm by adding miconazole powder for the prevention of dermatophytosis.

Nonhuman Primates: Prior to ordering, NHP’s health records are checked by DLAM veterinarian, then, and based on standard veterinary practices and study needs, a tailored preventive program is designed for additional diagnostics tests and preventive treatment with vaccinations and antiparasitics. At receiving all NHP received a physical examination then at least annually. Nails are checked at least monthly and trimmed as needed. Weight is taken upon receipt and at least once monthly. All NHPs are tested for TB at least twice a year and Herpes B virus at least once annually. Dental prophylaxis is performed as needed per Veterinary discretion. Older animals (typically greater than eight years of age) may receive semiannual physical exams, hematology, and clinical chemistries.

Gerbils and Hamsters: Gerbils are weighed monthly and monitored daily for health and any significant weight loss or health concerns are reported to the veterinarian. Toenails are inspected each month and trimmed if needed.

Pigeons: The pigeon colony has been closed since 2009. Sentinel animals are not in place. Any animal that has been euthanized or found dead has been submitted for complete necropsy and parasitology testing for “herd health” management.

Guinea pigs: Guinea pigs are weighed monthly, and any significant weight loss is reported to the veterinarian. Guinea pigs are received from SPF vendors.

Lamprey: The source for these animals is a collaborator of the PI and has no health history; there is no sentinel system for these animals. Animals are examined at receipt and monitored daily for health. Any found dead would be considered for complete necropsy / sample collection at the discretion of the veterinarian for a

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“herd health” management standpoint. Chickens (as chicks): Chicks are ordered from a DLAM-approved vendor and

examined at receipt. Any found dead during the short course of the experiment would be subject to a full necropsy and collection of samples for testing at the discretion of the veterinarian for a “herd health” management standpoint.

Fish (Zebrafish and other spp.): Fish are either imported to UCLA from collaborating institutions or purchased from reputable exotic animal dealers or pet stores (such as Petsmart). There is typically no medical history submitted to DLAM veterinary staff from these sources unless they are coming through the formal import process. Animals are examined by laboratory staff and veterinary staff on an as-needed basis on arrival. Preliminary sentinel testing of sump fish from the zebrafish Core have all tested negative for zebrafish pathogens of concern. A regular sentinel testing program for these fish and other zebrafish housing areas is being finalized.

Salamanders, Toads, Axolotls, Newts: As these animals are typically obtained from non-DLAM approved vendors (reputable exotic animal dealers or pet stores), there is no health history. There is no sentinel program in place. Any animal found dead would be subject to a full necropsy and collection of samples for testing at the discretion of the veterinarian for a “herd health” management standpoint.

Birds (Zebra finches): All finch colonies have been closed for several years. There is no sentinel program in place. Any found dead would be subject to a full necropsy and collection of samples for testing at the discretion of the veterinarian for a “herd health” management standpoint.

Bats: No sentinel testing program is in place. There is no vendor surveillance available for the sources of these two species. Any animal found dead or euthanized for which the brain is not required for tissue collection is submitted intact to the Los Angeles County Health Department for rabies testing. No animals have ever tested positive.

2. Emergency Care [Guide, p. 114]

a. Describe the procedures to ensure that emergency veterinary care is continuously available for animals during and outside of regular work hours, including access to drugs or other therapeutics and equipment.

In the event of an animal health emergency during regular work hours, the veterinarian on-duty is available by contacting the DLAM phone tree or the veterinarian cell phone directly. DLAM veterinarians provide after-hours coverage on a rotating basis, although the clinical veterinarian (Dr. Torres) provides most of the after-hours coverage on a regular basis. A veterinarian can be reached at all times by calling the phone tree number, which will direct them to the person that is on call. Appropriate signage for after hour emergency care is posted in the animal facility, in all study areas, and on DLAM’s website. This information is also provided during research animal training. The on-call veterinarian has access at all times to necessary drugs, therapeutics and equipment.

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b. Describe the authority of the Attending Veterinarian or his/her designee relative to the emergency treatment of animals in the program.

In the event of an animal emergency, the Attending Veterinarian (AV) or designee (often the on-call veterinarian or after-hours veterinary staff) has ultimate authority (See the ARC Policy on Authority of the Attending Veterinarian; http://ora.research.ucla.edu/RSAWA/ARC/Pages/ARC-policies/attending-veterinarian.aspx). The veterinary staff and/or on-call veterinarian will assess the animal and attempt to contact the investigator, so that options for treatment or euthanasia can be discussed and offered. If the PI cannot be reached within a reasonable timeframe, the veterinary staff will exercise their clinical judgment with the welfare of the animal as the highest priority. For covered species, treatment is more often elected and all treatments are recorded.

3. Clinical Record Keeping [Guide, p. 115]

a. Describe the procedure for maintaining medical records and documenting treatment of ill animals including: clinical laboratory findings, diagnoses, treatments, medical progress records, etc. Identify the species for which individual records are maintained and where such records are kept.

Active Medical records, including clinical laboratory findings, diagnoses, treatments, and medical progress for all USDA-covered species are archived in the DLAM Surgical office (CHS 2V-124) by the veterinary technicians. When needed, medical records are maintained in the animal room (while a clinical case or post-procedural care remains open). Individual records are maintained for NHPs, Swine, chinchillas and rabbits. The rest of the USDA-covered species (e.g. hamsters, bats, etc.) generally have group records. Medical records are established per veterinary discretion and include but are not limited to: Species, weight, gender, identification, and Animal Use protocol number History or information as it pertains to each animal's medical status. Data collected during physical examination Procedure records and reference to research interventions when appropriate.

Surgery, anesthesia, analgesia, and peri/post-operative care. Treatment and intended treatment plan, including medications, their dosage and

frequency of use All medications and treatments prescribed and dispensed Documentation provided by the vendor Only abnormal findings, daily progress, and disposition of case. Behavioral and

individual animal enrichment notes. Euthanasia and other dispositions and necropsy findings if indicated.

For mice and rats, information regarding the room, rack, cage, protocol, and PI is entered into our web-based program (REACTOR). This information becomes

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instantaneously available to the veterinarian reviewing clinical cases. This health reporting system is complemented by a quick electronic notification system, which automatically incorporates relevant information, including an action deadline, into an e-mail message that is sent to the research laboratories. The investigator can then respond to the health case notification directly via the web site. This response becomes visible to all DLAM veterinarians and animal health technicians. If treatment is an available option, and the investigator decides to treat, he/she is responsible for entering all treatment information on a treatment card that is placed behind the regular cage card, unless arrangements have been made with DLAM staff to do this. If no treatment or response from PI at the end of the deadline, DLAM will treat or euthanize the animal.

b. Identify individual(s) (titles, not necessarily names) responsible for maintaining such records and identify where the records are maintained and who, including the IACUC/OB has access to the records.

Veterinary staff and/or researchers are responsible for maintaining medical records. For USDA-covered species, medical records are maintained in the animal holding room and available for animal care, veterinary and research staff with access to that room. Medical information in REACTOR is available to veterinary and research staff. Medical information is available to the ARC upon request at any time.

c. Describe the role of the Attending Veterinarian in recordkeeping.

The AV, or designee, is responsible for ensuring that appropriate medical records are initiated, maintained and kept for all animals on campus including PI-maintained animals in study areas (e.g. bats).

4. Diagnostic Resources. Describe available diagnostic methods used in the program including:

a. In-house diagnostic laboratory capabilities.

Specimen storage: In house specimen storage capability includes refrigeration, -20° and -80° freezers.

Hematology: Routine and stat hematology specimen testing is performed in house on a Genesis Multi-species hematology analyzer. Oxford Science controls are used. Confirmatory hematology tests if necessary may be to a veterinary reference laboratory (IDEXX).

Chemistry: Routine and stat serum/plasma chemistries are performed in house on an Alfa Wasserman Vet Ace VetAxcel chemistry analyzer. Alfa Wasserman GEMCAL calibrator, CO2 Standard, and QC1 (normal) and QC2 (abnormal) control sera are used. Non- routine chemistries are sent to a veterinary reference laboratory (IDEXX).

Parasitology: All routine parasitology is performed in-houseRoutine fecals are 121

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processed using a formol-ethyl acetate concentration method and are evaluated in the lab.

o Routine fecals are processed using a formol-ethyl acetate concentration method and are evaluated in the lab.

o Cellophane tape preparations on rodents are examined for Syphacia spp. Ova and fur mites.

o Cellophane tape preparations, skin scrapings, hair pulls, pelts, and other specimen are examined for ectoparasites.

o Intact adult parasites are identified microscopically.o Cecal contents of Sentinel animals are examined under a dissecting scope

for adult pinworms.o In-house consultation with the parasitologist for the UCLA, School of

Public Health, is also available. Urinalysis: Performed using Multistix 10SG (Bayer) reagent strips and microscopic

examination of urine sediment. Chek-Stix (Bayer) positive and negative control strips may be used.

Mycology: Routine mycology is submitted to a veterinary reference laboratory (IDEXX).

Bacteriology: Routine bacteriology is submitted to a veterinary reference laboratory. Contact plates with DE Neutralizing agar are used for environmental testing (cage washer) and are incubated and counted in-house.

Serology: Routine rodent serology (Multiplex Fluorescent ImmunoAssay; MFIA) is performed in- house using IDEXX BioResearch reagents and controls. MFIAs are performed using BioRad equipment and Bio Rad software. Confirmatory testing and individual tests may be submitted to Charles River, or IDEXX BioResearch.

PCR: Routine PCR (e.g. for Helicobacter and Mouse Parvovirus) is conducted in-house or sent to IDEXX BioResearch or to Charles River labs.

Cytology: Routine cytology is stained in- house with Wright-Giemsa, Diff-Quik, or Gram Stain. Cytology specimens are read by a contracted veterinary pathologist.

Histopathology: Tissues for slide preparation are sent to UCLA TPCL (Translational Pathology Core Lab) Histology Lab, in-house DLAM histocore, or outsourced to UC Davis or IDEXX BioResearch. Tissues are sectioned and interpreted by a contracted veterinary pathologist.

b. Commercially provided diagnostic laboratory services.

Commercially provided diagnostic laboratory services are obtained from the laboratories listed in the key below. All specimens are prepared and packaged for shipment in compliance with Department of Transportation (DOT) regulations. In addition, the DORA (Directory of Rare Analysis) is used as a reference to locatelaboratories that perform non-routine tests.Laboratory TestCharles River Lab Serology confirmation, Molecular

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251 Ballardvale StreetWilmington, MA 01887(800)338-9680

Diagnostics Rodent PCR

IDEXX CA 1370 Reynolds Ave, Suite 109Irvine, CA 92614(800)444-4210

Clinical diagnostics, Histology, Molecular Diagnostics Rodent PCR

IDEXX BioResearch4011 Discovery DriveColumbia, MO 65201

Serology, rodent PCR

Iowa State U. Diagnostic Lab 1600 S. 16th St.Ames, IA 50011(515)294-1950

Pig Serology

LabCorp 1904 Alexander DriveResearch Triangle Park, NC 27709(919)572-7544

T3, T4, PTH, TSH samples

NIH B Virus Resource Laboratory 50 Decatur StreetAtlanta, Georgia 30303(404)651-0808

All B Virus specimens

UCD Comparative Pathology Lab Old Davis Road, Bldg. R-1Davis, CA 95616-8520(530)752-2832

Histology

USDA- National Veterinary Services Lab Ames, IA 50010(515)239-8200

Swine disease tests

c. Necropsy facilities and histopathology capabilities.

The necropsy room is located on the 5th floor of the CHS vivarium. It consists of a 256-ft2 main necropsy room and a 94-ft2 adjoining room. The main necropsy room contains two Hamilton fume hoods for pouring formalin, preparation of sections and decalcification, for bagging tissues to be returned to investigators and animal perfusions. The necropsy room and the anteroom each contain a down draft/back draft charcoal-filtered tissue sectioning table (Mopec). The necropsy table is suitable for the necropsy of animals ranging in size from mice to average sized swine. The room features specialized equipment for the collection of tissues and measuring of organ weights, a striker saw to cut through bone for removal of brains from medium and large size animals, and Scout Proscales and Pioneer precision scales for measuring the organ weight of mice for phenotypic analysis.

Currently, all tissues are sectioned on downdraft or backdraft charcoal filtered tissue 123

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sectioning tables and are sent to the UCLA TPCL (Translational Pathology Core Lab), or two outside labs (UC Davis and IDEXX BioResearch) for paraffin embedding, sectioning and staining. These labs have a 7-day turnaround time for both H&E tissue section staining as well as for special stains. For frozen tissues sections and for rapid (24-48 hr) turnaround times, we use the UCLA TPCL (Translational Pathology Core Lab). We currently also have an in-house (DLAM) histology core that is being utilized for low-volume sample processing. Cytologic samples are stained in our facility using the Wright-Giemsa and Gram stain methods.

Necropsy and cytologic reports are completed and stored in the Sirius database. Reports can be printed from this program and the files can be stored for subsequent retrieval. The database also allows for information searching during retrospective studies.

d. Radiology and other imaging capabilities.

Radiology, fluoroscopy, computed tomography, ultrasound, and magnetic resonance imaging are all readily available in the Translational Research Imaging Center (TRIC) and Lab Rigler Center, an integrated research area for interventional radiology studies and for health cases (typically large animal) if needed.

For rats and mice, the California NanoSystems Institute (CNSI) at UCLA provides microCT, PET and optical imaging capabilities that are typically for research purposes but could be used for diagnostics if needed.

For rats and mice, an investigator-maintained Faxitron imaging device is available in his laboratory space that might be used for clinical imaging on an as-needed basis.

5. Drug Storage and Control

a. Describe the purchase and storage of controlled and non-controlled drugs.

Non-controlled drugs are ordered and received by DLAM personnel and are stored in the DLAM pharmacy in the CHS building (6V), health clinic cabinets or refrigerator, per the pharmaceutical requirements.

Controlled substances are ordered through the UCLA Pharmacy Vault by DLAM Veterinary Staff and stored in the DLAM pharmacy in a double-locked stainless steel cabinet. Controlled drugs that need refrigeration are kept in a double-locked cabinet in the refrigerator of the CHS, 8V clinic.

The ARC monitors proper storage of controlled substances maintained in DLAM and in PI labs during semi-annual inspections of those areas. PIs must procure controlled substances from the university hospital pharmacy Vault, and maintain the required forms for use of these substances in their own studies; DLAM cannot dispense these

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drugs.

Institutional minimum requirements for the storage of controlled substances include: A securely locked, substantially constructed cabinet with no sign or any other indication that the cabinet is used for the storage of controlled substances. Cabinets constructed of materials that are fragile and/or allow visualization, such as glass or plastic, are considered inappropriate for this purpose.

It is recommended that entry doors to the area where controlled substances are stored be off master key systems, where practical. If a keyed lock is used, the key shall be kept in a location separate from the storage cabinet. Keys are to be carried by authorized personnel or in a locked container/room that is restricted to authorized personnel. Combinations are accessible to authorized personnel only.

The required Controlled Substance Disposition Record(s) must be maintained and available during regular business hours to representatives of the ARC, the Attending Veterinarian, University of California officials, and regulatory or accreditation agencies.

Expired controlled substances obtained from the UCLA Pharmacy must be labeled as such returned to the UCLA Pharmacy together with the corresponding disposition record(s). The supplier of non-UCLA Pharmacy obtained drugs must be contacted for disposal instructions, if needed. Records of controlled drug procurement, storage, use and disposition are reviewed during facility inspections.

b. Describe record keeping procedures for controlled substances.

A log for controlled substances used by DLAM is maintained in the controlled substances cabinet in the DLAM CHS surgical suite. Exact volumes removed from the bottle are recorded on the corresponding sheet and subtracted from the previous subtotaled volume. DLAM Executive Director or designee personally inspects and signs off on all controlled substance records before these are returned to the UCLA Pharmacy Vault. Investigators are also required by the IACUC to keep accurate records and keep all drugs locked in a secure place in their laboratories. The IACUC Policy “Storage of Controlled Substances” is used as a guide for proper storage of these drugs.

D. Surgery [Guide, pp. 115-123]

1. Pre-Surgical Planning [Guide, p. 116]Describe the process(es) used to ensure adequate pre-surgical planning, including: identifying personnel; locating equipment, supplies, veterinary involvement for selecting analgesic and anesthetic agents and facilities; planning; and pre- and post-operative care.

All personnel involved in surgical procedures are initially identified in the investigator’s 125

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animal use protocol. Surgical procedures are specified and detailed in the protocol. At the time of veterinary pre-review of all new, renewal and amendment protocols, a veterinarian may give advice or suggestions regarding any aspect of the surgical procedure, anesthesia and analgesia and post-operative care. The DLAM and ARC websites also contain information on surgery policies and procedures including record-keeping. New animal users must take surgery and pain and distress modules in CITI and attend a training class on Aseptic Surgical preparation, which is held at least weekly in the CHS training facility. Investigators planning on using the CHS 2nd or 5th floor suites for rodent surgeries are given an orientation and overview prior to their first procedure, including written instructions on the proper use of this area, a sample surgery record/post-op log and a rodent surgery checklist. A DLAM veterinarian is always present for the first USDA-covered species surgeries performed by a new research group. Often, if the ARC has questions on any surgical procedures, they may require (via ARC codicil) that a DLAM veterinarian be consulted or be present the first time this procedure is conducted, regardless of species.

DLAM manages and operates the central surgical facility (CHS, 2nd floor) designated to be used for USDA covered species. A veterinarian from DLAM meets with new investigators to discuss pre- and post-op procedures, as well as anesthesia, analgesia, and aseptic technique. The veterinarian or a qualified technician oversees the procedures being performed according to the approved protocol and observing proper aseptic, anesthetic, surgical techniques), and perform or supervise post-operative care.

The Translational Research Imaging Center (TRIC) is an interventional radiology experimental area operated by the Department of Radiological Sciences. The TRIC manager meets with investigators to schedule procedures and ensure that all required equipment and supplies are available. Technicians employed by the Department of Radiological Sciences assist in anesthesia monitoring and non-survival surgical procedures. Recovery surgeries are performed in the DLAM Surgery suite (CHS, 2nd floor).

The surgical facility in NRB is part of the Fuster Laboratories in Cognitive Neuroscience designated to be used for NHP and is operated and managed by the research lab manager and DLAM personnel hired by the lab. The lab manager, PI, and DLAM personnel communicate to establish scheduling of procedures. The Surgery Manager helps to identify DLAM personnel who will participate. The lab manager and DLAM personnel work together to locate equipment and supplies, pre-surgical planning, and in some cases, pre-operative care. DLAM either performs, or provides oversight for postoperative care.

The Laryngeal Lab surgery room (CHS) is ARC-approved for non-survival dog surgeries and survival surgery of chinchillas and mice. The investigator’s technicians and residents oversee the logistics and surgical monitoring in his area. Observation of procedures by veterinary staff confirms that the personnel involved are competent to perform the procedures and successfully administer and monitor anesthesia. DLAM veterinary staff provides direct oversight of post-operative care.

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DLAM maintains surgery suites for survival procedures on non-USDA-covered species (rodents) in CHS (2nd and 5th floors). The 5th floor suite consists of a large surgery area (312 ft2), with five fold-down surgical tables, and a smaller prep room (72 ft2) equipped with oxygen, an isoflurane anesthetic machine and a functional sink. This prep room is used for anesthetic induction and pre-surgical preparation of animals and surgeons. The main surgery room features isoflurane vaporizers, connected to a central oxygen supply source; overhead surgical lights; backup emergency lighting; water-circulating heating pads; and glass-bead sterilizers. The 2nd floor suite is similarly instrumented but smaller, and has 5 surgical tables. The individual labs using these suites are responsible for providing all other equipment and supplies needed for their specific procedures (including instruments and drapes). Day-to-day operation of this room is overseen by a qualified DLAM veterinary technician, who provides advice and assistance as needed. Postoperative monitoring is typically provided by the research labs. The ARC recommends the use of this surgical area to all labs performing survival mouse and/or rat surgery, unless use of it would be impractical for their studies (such as requiring a large piece of sensitive equipment that cannot be transported to and from this room).

2. Surgical Facilities [Guide, pp. 116-117, 144-145]List building name(s) and room number(s) or other locations (coded, if confidential) where surgical procedures are performed. For each, describe:

the type of species (including rodents, fish, agricultural species, etc.) nature of procedure(s) (major/minor/emergency, survival and non-survival,

etc.) the amount of use [heavy (daily), moderate (weekly), or light] major surgical support equipment available (gas anesthesia machines,

respirators, surgical lights, etc.) facilities for aseptic surgery, surgical support, animal preparation, surgeon’s

scrub, operating room, and postoperative recovery construction features of the operating room(s), including interior surfaces,

ventilation, lighting, and fixed equipment used to support surgical procedures and other means of enhancing contamination control

Note: If preferred, the information requested in this section may be provided in Table.

The animal surgical program at UCLA can be divided into two types of programs-those that are DLAM-managed or Joint DLAM-PI managed and present within the DLAM vivaria, and those that are managed and overseen by individual and independent researcher labs and are found either inside or outside the DLAM vivaria:

DLAM-managed and Joint DLAM-PI managed surgical programs include those that are operated in surgical facilities on the 2nd floor of the CHS vivaria (for USDA-covered species), 2nd and 5th floors of the CHS vivaria (for non-USDA-covered species, primarily mice and rats), B floor of CHS (TRIC lab; primarily USDA-covered species),

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and 5th floor of NRB (NHP). In these areas, DLAM veterinary presence is constant, and involves performing some aspects of the procedure such as preparation, anesthesia, recovery, and/or post-operative care. It also involves one on one continuous training of laboratory members who will be conducting the studies. A list and details of these facilities are found in Appendix 24.

Investigator-managed surgery areas for USDA-covered species, are utilized mainly for non survival procedures. They are equipped with appropriate anesthetic systems, based on species and type of procedure e.g. pigs vs chinchillas, cardiac electro- physiology vs laryngeal physiology. For survival procedures, a separate space for preparation of the animals is required. Isoflurane is the main anesthetic agent and most areas are equipped with anesthetic machines and mechanical ventilators, as well as temperature support devices and devices for fluid administration. Frequently, DLAM veterinary staff have some involvement with the surgeries in these areas such as responsibilities for post-op care or constant oversight and review of records and record-keeping. Investigator-managed rodent surgery areas vary in size and location, as well as in equipment. The minimum equipment required, when using volatile anesthetics is: source of oxygen, anesthetic vaporizer, induction chamber, anesthetic system, scavenging system for volatile anesthetic waste, and heat support. This equipment, including its maintenance, and surgical programs, records, etc. are inspected during ARC semiannual facility inspections. A list and details of these facilities are found in Appendix 25.

3. Surgical Procedures [Guide, pp. 117-118]

a. Describe the criteria used to differentiate major from minor survival surgery, including classification for certain procedures (e.g., laparoscopic technique).

Major surgery is defined as any surgical intervention that penetrates an exposes a body cavity, produces substantial impairment of physical or physiological functions, or involves extensive tissue dissection or transection. Examples of major surgery include laparotomy, thoracotomy, craniotomy, joint or bone replacement, spinal transection, and limb amputation. Minor survival surgery does not expose a body cavity and causes little or no physical impairment. Laparoscopic and other percutaneous techniques are categorized as major or minor depending on the potential for pain and other intra or post-operative complications (e.g. bleeding); the nature and duration of the procedure as well as the species, health status, and age of the animal. For example, myocardial infarcts created via percutaneous endovascular catheters are considered major surgeries. Procedures are evaluated on a case-by-case basis by the veterinarian and the ARC.

b. How is non-survival surgery defined?

Non-survival (Terminal) surgery is defined as a surgical procedure from which an animal is euthanatized, for scientific and/or human reasons, before recovery from anesthesia. This definition does not include animals that are euthanized due to

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intraoperative complications that cannot be resolved with veterinary intervention.

4. Aseptic Technique [Guide, pp. 118-119]

a. Describe procedures, equipment, and protective clothing used for aseptic surgery. Include patient and surgeon preparation.

Survival surgery must be performed using aseptic techniques. The ARC and DLAM veterinarians have developed aseptic surgery guidelines http://ora.research.ucla.edu/OARO/Pages/ARC-policies/mice-rats-birds-surgery.aspx, which are incorporated into the ARC protocol and/or posted on the ARC website. This includes performing the surgery in a dedicated space, removal of hair, cleaning and disinfecting the surgical site, usage of sterile gloves and instruments, and adherence to appropriate technique during surgery. The investigator is responsible for supervising the surgical procedure and providing, or coordinating with DLAM for, adequate support staff, instruments, supplies and drugs. Major survival surgical procedures in USDA-covered species are conducted in dedicated surgical suites intended for that purpose, maintained and operated under aseptic conditions. Surgery on rodents does not require a dedicated surgical suite but instead an appropriate area dedicated at the time of the surgical procedures. DLAM provides training in aseptic surgical technique which is an ARC requirement for any researcher performing surgery.

b. Describe methods used to sterilize instruments and protective clothing, including a description of approved liquid sterilants and instrument exposure time(s) required for each, if applicable.

Methods used to sterilize instruments and other equipment include autoclaving, gas sterilization, chemical sterilization, and dry heat (e.g. hot bead sterilizer). Sterile disposable supplies such as disposable sterile gowns and surgical gloves, percutaneous needles, catheters & guide wires are pre-packaged and used for survival procedures. Reusable supplies are placed in sterilization pouches with color change indicators and sterilized by either heat (steam autoclave) or gas (ethylene oxide; EtO) exposure. Commercially sterilized items are considered sterile until the expiration date on the package. In house sterilized items have the sterilization date written on the package and are considered sterile for up to six months. Because of its physical properties some materials cannot be sterilized with heat or gas, therefore the ARC has approved the use of chemical sterilants. SOPs should be issued by the lab and approved by EH&S and/or ARC to describe these procedures. From Table 2: Recommended Methods of Instrument Sterilization on the ARC policy website (http://ora.research.ucla.edu/OARO/Pages/ARC-policies/mice-rats-birds-surgery.aspx):Agents Examples CommentsPhysical:Steam sterilization (moist heat)

Autoclave Effectiveness dependent upon temperature, pressure and time (e.g., 121.6°C for 15 min. vs. 131°C for 3 min.).

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Chemical:Gas sterilization

Ethylene Oxide

Requires 30% or greater relative humidity for effectiveness against spores. Gas is irritating to tissue; all materials require safe airing time. Carcinogenic. Suitable for catheters and implants.

Chlorine Dioxide

Clidox®, Alcide®

A minimum of 6 hours required for sterilization. Corrosive. Presence of organic matter reduces activity. Chlorine-based disinfectants must be fresh (<14 days). Must be thoroughly rinsed from instruments using sterile distilled water before use.

Aldehydes Gluteraldehyde Many hours required for sterilization. Corrosive and irritating. Consult Biosafety Officer on proper use. Must be thoroughly rinsed from instruments using sterile distilled water before use.

Dry heat: Hot bead sterilizer

Fast (15 to 20 seconds). Instruments must be cooled before contacting tissue. Instruments must be sterilized by one of the above methods prior to first use that day.

c. Describe methods for instrument re-sterilization between serial surgeries.

For rodents, surgical instruments may be used on more than one animal; however, any item intended to be used on multiple animals must be first sterilized by one of the methods mentioned in item D.4.b above and then carefully cleaned and sterilized between animals. Hot bead sterilizers are preferred for tip sterilization; users must ensure that all blood/tissue debris is wiped from the instrument tip(s) before insertion into the glass beads. Rodent surgery suites managed by DLAM are equipped with hot bead sterilizers for investigator’s use.

d. Indicate how effectiveness of sterilization is monitored.

Temperature indicator strips are used to verify the autoclave reaches the temperature necessary for heat sterilization. EtO gas dosimeters are used to verify the EtO gas sterilizer reached the designated EO gas concentration necessary for gas sterilization. Sterilization records are maintained by the operator of the equipment. All autoclaves managed by DLAM, are monitored quarterly by the use of spore tests that are submitted to the DLAM diagnostic lab for developing the reaction and final reading. For hot bead sterilizers, based on manufacturer’s recommendation, beads are replaced every 6 months. The EtO sterilizer receives bi-annual QC leak tests performed by an outside vendor. Records for the EtO gas sterilizer are maintained by the Fuster Laboratories in Cognitive Neuroscience.

e. Describe surgical support functions provided by the program to investigators.

Main Surgery Suite for Covered Species (2V-124 suite): In this area DLAM provides patient prep, anesthesia, surgical support and recovery procedures (as needed) to investigators scheduled to use this core facilities. The suite is divided in different areas

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including prep room, regular surgery suites and a hazardous surgery suite. This facility is equipped with multiple anesthetic systems, including mechanical ventilation, as well as with monitoring and support equipment. (See Appendix 24 for details)

Rodent surgery suite managed by DLAM (2V-125) patient prep, anesthesia, surgery support and recovery is available for investigators. The room has a prep area and a common surgical area with 5 tables. Each table is equipped with an isoflurane vaporizer, a water circulating pump and surgical light. There is a hot bead sterilizer available in this room. (See Appendix 24 for details)

An autoclave for surgical instruments sterilization is located in CHS 2V-213A. This equipment is maintained and operated by DLAM, It is used for the surgical equipment utilize for covered species as well as to provide autoclave services for investigators conducting surgery outside the DLAM suites.

The TRIC Lab (BV-135, BV-227, BS-261A) technicians provide patient prep, anesthesia, radiology support and recovery procedures (as required) to each investigator scheduled to use the lab. Patient prep and recovery can be performed in either BV-135, or BV-227. BV-121 is available for post procedure recovery for animals after major procedures (e.g. myocardial infarcts). Surgical instruments used in TRIC are autoclaved by DLAM. For other equipment, see Appendix 24.

NRB Main Surgery Suite (Fuster): Room 520M is used for instrument cleaning including a sink and pack preparation. The autoclave is located in 520N. The surgeon’s scrub area is located in 520N. The patient prep area is 520M.

5. Intraoperative Monitoring [Guide, p. 119]Describe monitoring and recording requirements for each species, including the type of record(s) maintained. Also note monitoring of anesthesia during non-survival procedures.

Any surgical procedure lasting between 15 and 30 minutes or non-surgical procedures requiring no more than one injection of a short acting anesthetic require: Continuous visual confirmation of normal respiration with the respiratory rate recorded

every 15 minutes Intermittent heart auscultation or pulse palpation with the heart rate/pulse rate recorded

every 15 minutes For non-rodents, body temperature every 15 minutes until the animal is sitting or

standing up For rodents or similarly sized animals, cages may be partially placed on a safe heat

source. Hazardous animals, such as NHPs, are returned to their home or transport cage for

recovery and continuously monitored until they are conscious and sitting up. Respiratory rate and pattern are monitored and may be recorded from outside the cage, but pulse rates and thermometry are not necessary.

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For procedures over 30 minutes on non-rodent species: Continuous visual confirmation of respiration with respiratory rate recorded every 15

minutes. Capnography is required for all major survival and non-survival surgery in USDA

covered species, when the animals are endotracheally intubated. It should be continuously assessed and recorded every 15 minutes.

Continuous pulse oximetry with heart rate and SpO2 recorded every 15 minutes.. Body temperature is recorded every 15 minutes.

6. Postoperative Care [Guide, pp. 119-120]Describe the postoperative care program, including who is responsible for overseeing and providing the care, types of records maintained (e.g., perioperative), where the records are maintained, etc.

For USDA-covered species, a DLAM surgery technician, a member of the PI’s staff, a qualified technician, or a veterinarian continuously monitors each animal until it is conscious and sternal. During this time, notations are made regarding the animal’s recovery every 15-30 minutes in the postoperative record. Temperature, pulse and respiration must be recorded at least every 15 minutes until the animal is conscious and sternal. Animals undergoing more complex procedures are monitored more intensively according to protocol instructions. After the animals are sternal and conscious, they may be returned to their cages. However, most animals are monitored intermittently until they are walking.

The first dose of analgesic medication, if not given pre-emptively before surgery, is administered at approximately the time of extubation. For covered species in category D protocols, analgesic medication is given as described in the ARC protocol and generally continued for 48 hours post-operatively, and 24 hours for minor surgeries, and for as long as necessary if the animals are exhibiting signs of pain.

A veterinarian or qualified technician performs a physical exam and pain assessment on each post-surgical patient at least once daily for one day after anesthetic recovery (and, also on the afternoon of anesthetic recovery) and then continues to monitor for at least the first 48 hrs. post-operatively, including weekends and holidays. Monitoring of the surgical site, appetite, signs of pain/distress, and general health are expected during this period. For many procedures, a surgical technician and/or the PI’s staff continues monitoring according to protocol instructions.

All post-operative observations and actions are recorded in the animal’s individual record directly, or on the post-operative sheet, which is placed in the animal’s individual record after the post-operative period has ended. The veterinary staff monitors the post-operative records for all surgical procedures.

For mice and rats, the investigator’s laboratory staff is responsible for monitoring the 132

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animals after surgery, as well as administering all analgesics and antibiotics as per their approved animal use protocol. DLAM technicians also provide this service when needed. Following surgery, all animals are checked at least daily, by lab staff during the post-op period. Records are kept either in the room where the animal is housed after recovery from surgery, or in the investigator’s laboratory. A veterinarian may request to review this information at any time. A sample sheet for the labs to use to record treatments and observations is provided to them. Additionally, a post-op sticker is required by the ARC to be placed on the cage card of every post-op mouse or rat, indicating the procedure performed; the date; the name and dose of post-op medications (such as analgesics and antibiotics); the date and time of their administration; and the contact name and phone number of the staff member responsible for the animals. The day following surgery, the animal is checked by DLAM animal care staff as part of regular daily monitoring, and any abnormalities brought to the attention of the veterinary technicians or the veterinary staff. Repeated or serious problems (such as wound dehiscence or failure to administer analgesics on-time) result in a discussion between a veterinarian and the PI or lab staff to resolve the problem. Whenever a negative pattern is identified, the deviation is also reported to the ARC.

E. Pain and Distress [Guide, pp. 120-121]

1. Describe how and by whom pain and distress are assessed.

The potential for pain and distress is discussed with each investigator at the time of initial veterinary review of the proposed animal use protocol. The assumption is made that any procedure likely to cause pain in humans is also likely to cause pain in animals. The ARC follows the USDA Animal Welfare Regulations and categorizes the pain levels as C: minimal pain or distress (i.e., an injection), D: potential for pain and distress relieved by analgesia (i.e., most surgical procedures), or E: potential pain and distress unrelieved by analgesia but scientifically justified. For procedures that may cause pain or distress, the frequency of observation, post-procedure, is determined in the protocol and/or by the veterinarian based on the invasiveness of the procedure (including surgical and non-surgical), and other risks for pain and distress. Immediately after procedures, animals are continuously observed by the research and/or veterinary staff for signs or pain and distress. These observations sometimes go for long periods of time, for example hours in covered species after long major procedures, and rodents after injection of substances of unknown toxicity; or for short periods of time until the animal is ambulating if the procedures are short and minor. After this initial stage, animals are then observed at least daily for a few days up to the duration of the study.

Once the protocol is approved, animals are ordered and potentially painful procedures are performed, pain and distress are assessed by trained DLAM staff at least daily in DLAM-managed areas. Again, additional observations by research staff are dictated by the ARC protocol. DLAM husbandry technicians are trained on abnormal behavior/postures that may indicate pain and/or distress. If an animal is found having these characteristics, it is brought to the attention of the veterinary technicians.

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2. Describe training programs for personnel responsible for monitoring animal well-being, including species-specific behavioral manifestations as indicators of pain and distress.

DLAM employees receive training in identification of normal behaviors and healthy appearance of the different species they work with, as well as recognition of pain and distress. This training is based on the HERSLAW model, which systematically assesses the animals. These topics are taught in different scenarios such as departmental SOP training, on the job training, and All Staff meetings (taught here annually).

For investigators, the ARC requires species specific classes which are taught by experienced veterinary technicians and veterinarians and include normal behaviors and appearance of the particular species, as well as how to report abnormal conditions to the veterinary staff. There are also CITI modules, mandated by the ARC that involve these topics such as animal species-specific courses, and post procedure care of mice and rats in research: minimizing pain and distress; the latest includes the module systematic monitoring of pain and distress.

In addition, an annual class is offered to the research community to discuss abnormal conditions in mice and rats, this class is taught by DLAM veterinarians. Attendance by staff responsible for animal care in study areas is required. On-going training in animal care is provided on a one-on-one basis when health check visits are made to the study areas by the veterinary technicians or the veterinarian.

All investigators and lab members working with covered species receive one-on-one training on recognition of pain and distress, from DLAM veterinarians and veterinary technicians, during the conduct of their experiments.

F. Anesthesia and Analgesia [Guide, pp. 121-123]

1. List the agents used for each species.Note: If preferred, this information may be provided in Table or additional Appendix.

Sedative, tranquilizer, anesthetics and analgesic drugs are provided in Appendix 26.

In addition to drugs, post-op animals may be provided with extra enrichment, in the form of (for rodents) extra nesting material to help them thermoregulate, or other enrichment in the cage (cardboard Shepherd shacks, plastic huts or tubes, etc.). Recovery cages are often placed half-on half-off heating pads as well. For rodents, water-moistened food pellets are often placed on the cage floor at surgery and the day after to encourage feeding. Larger species are kept warm during surgery and at recovery using Bair Huggers, as well as warm water and electric heating devices and pads.

When possible after surgery, animals are continued to be socially-housed; we teach 134

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research staff to use subcuticular suture patterns, so there are no exposed sutures for cage mates to chew out, so they can be recovered and housed again with their previous cage mates, which helps reduce stress, rather than singly-housing them for fear that partners will chew out sutures.

2. Describe how the veterinarian provides guidance and advice to researchers concerning choice and use of anesthetics, analgesics or other pain moderating methods.

A veterinarian pre-reviews any animal use protocol that involves more than slight or momentary pain or distress that will or will not be alleviated by sedatives, tranquilizers, analgesics or anesthetics. Analgesic and anesthetic choices are governed by the severity or invasiveness of the procedure and whether or not the drug will interfere with the investigators study. Any resistance to the use of the recommended analgesics or anesthetics must be justified.

3. Describe the monitoring of the effectiveness of analgesics, including who does the monitoring. Include in the description any non-pharmacologic means used to diminish pain and distress.

For USDA-covered species, a veterinarian or qualified veterinary/animal care technician examines all post procedural animals for signs of pain and/or distress and alters the regimen as needed per veterinary discretion. For rodents, the ARC will often recommend a first-time procedure be monitored by a veterinarian so that alterations in analgesic or anesthetic modalities can be made if needed. The ARC visits, semi-annually, investigators using anesthetics and analgesics, and examines stored drugs for expiration date and drug logs for evidence of use. Veterinary staff often interacts with the investigative staff and conducts routine lab visits during rounds or in response to an animal illness or injury report; this allows for additional monitoring of the use of anesthetics and analgesics

4. Describe how the veterinarian(s) and the IACUC/OB evaluate the proposed use of neuromuscular blocking agent to ensure the well-being of the animal.

The use of neuromuscular blocking agents is only approved for research procedures where scientific justification is provided for paralysis of the animal. Research staff are only allowed to use neuromuscular blocking agents under general anesthesia, and with appropriate monitoring, and prior evaluation according to ARC Policy (http://ora.research.ucla.edu/RSAWA/ARC/Pages/ARC-policies/neuromuscular.aspx ):

“Prior to using neuromuscular blocking drugs in a procedure, investigators must demonstrate to a DLAM veterinarian that the anesthetic technique is sufficient to prevent pain and distress associated with the procedure in the absence of the neuromuscular blocking agent, confirming that escape behavior does not occur.”

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“A surgical plane of anesthesia must be induced and the animal intubated prior to administration of the neuromuscular blocking drug; furthermore, unless described in an approved protocol, a surgical plane of anesthesia must be maintained during the entire time that the neuromuscular blocking drug is present and active in vivo. Neuromuscular blockers must not be administered until after the initiation of the surgical procedure (i.e., the skin incision) to ensure that the depth of anesthesia is adequate and the animal does not feel pain. Use of neuromuscular blocking agents should be confined solely to that phase of the procedure for which they are indicated. Neuromuscular blocking agents must not be used as a matter of convenience or to substitute for poor control of anesthesia.”

5. Describe policies and practices for maintaining and ensuring function of equipment used for anesthesia.

All precision anesthetic vaporizers owned by DLAM are maintained by a qualified anesthetic machine technician (e.g. Sierra Medical; Summit). The DLAM maintenance plan includes annual cleaning and basic maintenance, and triennial exchange for full maintenance and calibration. For PI-owned equipment, vaporizers must be tested at least once every three years by an authorized anesthetic machine service provider to verify accuracy of calibration. If the verified anesthetic delivery is > 10% out of calibration, the unit must be serviced by an authorized service provider. Vaporizers must have a certificate of the calibration date affixed directly to the machine/vaporizer after each service. In addition, a leak test must be performed by the lab at least annually.

G. Euthanasia [Guide, pp. 123-124]

1. Describe approved methods of euthanasia, including humane slaughter (for additional guidance, see pertinent AAALAC Reference Resources). Include:

consideration of species, age, condition (e.g., gestational period, or neonatal) and

location(s) for the conduct of the procedure.Note: If preferred, this information may be provided in Table or additional Appendix.

Methods of euthanasia are described in the ARC protocol and are consistent with the AVMA Guidelines for the Euthanasia of Animals (2013 Edition). The ARC has developed several policies on euthanasia including: Euthanasia of Rodents by Physical Methods Euthanasia of Fetuses and Neonates - Mice and Rats Rodent CO2 Euthanasia

To summarize, methods currently approved for non-regulated rodents are: Anesthetic overdose, followed by a physical confirmatory method CO2 inhalation, followed by a physical confirmatory method Decapitation (with or without prior anesthesia) Cervical dislocation (with or without prior anesthesia)

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Cardiac perfusion via non-survival surgery Microwave irradiation

The following locations have compressed CO2 gas cylinders with regulators, attached to a euthanasia chamber or to a cage lid that can be fitted onto an existing cage, that comply with AVMA guidelines:Building Room SystemBRI 12-399B ChamberBSRB B54A Cage Lid (mouse)BSRB B60B Cage Lid (mouse)BSRB B61H Automated system (Euthanex)BSRB B70H Cage Lid (mouse)CHS B1-266 ChamberCHS B6-085 ChamberCHS 1V-150 ChamberCHS 2V-520 Cage Lid (rat)CHS 3V-317 Cage Lid (mouse)CHS 3V-513 Cage Lid (rat)CHS 3V-526 Cage Lid (rat)CHS 3V-331 Cage Lid (mouse)CHS 3V-512 Cage Lid (mouse)CHS 3V-325 Cage Lid (mouse)CHS 4V-419 Automated system (Euthanex)CHS 5V-322/332 Chamber (mouse)CHS 5V-322/332 Chamber (rat)CHS 5V-335 Cage Lid (rat)CHS 6V-128 Cage Lid (mice)CHS 6V-133 Cage Lid (mice)CHS 6V-139 Cage Lid (mice)CHS 6V-323 Automated Thoren Euthanasia Rack system (mice)DEI 204F Cage Lid (rat)FH B404 Cage Lid (rat)Gonda 601 ChamberJSEI B114B Cage Lid (rat)LSB A914 ChamberMRL B225A ChamberNRB B05A Cage Lid (mouse)NRB B09G Cage Lid (mouse)NRB 320D Cage Lid (mouse)NRB 420A Cage Lid (mouse)TLSB B004 Cage Lid (rat)WH 21-132 Cage Lid (rat)/ Chamber

For USDA-regulated species, the method of euthanasia is determined in consultation withthe DLAM veterinary staff. Only non-physical methods are currently approved in regulated species. Pigs, rabbits, birds, NHPs and larger rodents are generally euthanized

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using pentobarbital-based products, often after initiation of anesthesia for a non-recovery surgery. Therefore, the location of euthanasia for these species could be anywhere, from the holding room to the surgery room, or any procedure location.

Aquatic animals are overdosed with MSS-222.

Euthanasia locations outside the vivaria (research lab locations) and euthanasia locations associated with non-survival surgery (within and outside the vivaria) are provided in Appendix 27.

2. Describe policies and practices for maintaining and ensuring function of equipment used for euthanasia.

The most common piece of equipment used is CO2 delivered from a compressed-gas canister. The canister has a regulator and flow valve attached with a tube that goes to either a chamber or can be directly attached to a ventilated mouse cage. This is provided, and regularly inspected and maintained by DLAM personnel.

Guillotines are also common used, and these are inspected regularly by the users and also by the ARC during the 6 facility inspections. The guillotines are mostly used after an animal is anesthetized or even commonly after death; only rarely are they used on an un-anesthetized mouse or rat. The ARC Policy on Euthanasia of Rodents by Physical Methods states the following: Recommendations of the AVMA Guidelines on Euthanasia state that “equipment used to perform decapitation should be maintained in good working order and serviced on a regular basis to ensure sharpness of blades.” Thus, prior to issuing approval for protocols listing decapitation as the method of euthanasia, the ARC now requires the following: 1) after each use, the unit should be wiped clean of any biological fluids to prevent buildup of potential corrosion; 2) after cleaning, a few drops of light machine oil (3 in 1) should be applied to blade surfaces and blade channels and the blades run together several times to spread the oil evenly over all moving surfaces. Blades should be replaced or sharpened regularly depending upon frequency of use. The ARC recommends the following technique to assess the sharpness of a guillotine: A guillotine is sharp enough if it will cut a thick rubber band, without dragging it between the blades and sticking.

3. Describe the methods used to confirm death of an animal.

The updated AVMA Guidelines for the Euthanasia of Animals: 2013 Edition emphasizes the need to confirm death following non-physical methods of euthanasia (i.e., CO2, anesthetic overdose). If vital organs (i.e., brain, heart or lungs) are harvested immediately after euthanasia, this is considered acceptable in lieu of a confirmatory method. Other confirmatory methods for commonly used species include the following: Mice: cervical dislocation, decapitation, thoracotomy Rats: decapitation, thoracotomy Rabbits: thoracotomy

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If one of these confirmatory methods will not be used, it is necessary to explain why in the approved ARC protocol, noting that animals must be observed for lack of a heartbeat and respiration and for graying of mucous membranes for at least 10 minutes to confirm death in order to comply with the Guidelines.

IV. Physical Plant [Guide, pp. 133-155]

A. Facilities Overview Provide a brief introduction to the animal housing and use facilities. Note that this overview should augment the information provided in Appendix 2 (Summary of Animal Housing and Support Sites), which includes area, average daily census, and person responsible for each site. Please use consistent terminology for the buildings/areas/sites described in the Location section of the Appendix. Please do not repeat information, but supplement the descriptions provided elsewhere to assist the reviewers understanding of the interaction between facilities, special housing locations, and separate procedural areas.

DLAM has active animal facilities in multiple buildings on and off the UCLA campus: three are connected within one large complex and generally referenced as CHS (BRI, CHS and Public Health); seven are located within one block of the CHS complex (BSRB, CNSI, Franz Hall, Gonda, TLSB, MRL, NRB); one is located one mile Southwest of the CHS complex (Warren Hall); and, one small rodent facility located off campus, 20 miles East of UCLA, within the USC Health Sciences Campus near downtown LA (Doheny). DLAM also has equipment storage space in 2 buildings (Rehab Center and Slichter Hall). There are 2 buildings formerly with vivarium space shut down for renovation (LSB and JSEI). These will no longer have central vivarium space when they reopen. Radiation Oncology is an independent vivarium located on the 6th floor of CHS vivarium tower. Information on Radiation Oncology is provided in Appendix 17 (study areas).

B. Centralized (Centrally-Managed) Animal Facility(ies) In this section, describe each centralized or centrally-managed animal housing and use facility. Include in Appendix 3 the floor plans of each on 8.5” x 11” or A4 paper. Ensure that the drawings are legible and the use of each room is indicated (animal housing, procedure room, clean cage storage, hazardous waste storage, etc.). Note that a separate section for describing “satellite housing areas” is included below.

Separately describe each Location or Animal Facility, addressing each of the features outlined below (1-8). A complete description of each must be provided; however, common features among locations or facilities may be indicated as such and do not need to be repeated.

1. General arrangement of the animal facilities (conventional, clean/dirty corridor, etc.).2. Physical relationship of the animal facilities to the research laboratories where

animals may be used.139

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3. Types of available animal housing spaces used, such as conventional, barrier, isolation/quarantine, hazard containment (infectious, radioactive, chemical), “animal cubicles” or facilities specifically designed for housing certain species such as ponds, pastures, feedlots, etc.

4. Finishes used throughout the animal facility for floors, walls, ceilings, doors, alleyways, gates, etc. (note any areas that are not easily sanitized and describe how these are maintained).

5. Engineering features (design, layout, special HVAC systems, noting exhaust air treatment, if applicable) used in hazardous agent containment.

6. Security features, such as control of entry, perimeter fences, gates, entryways, cameras, guards; identify and describe exceptions for individual facilities or areas incorporating fewer or additional security features than the general features described.

7. Consideration for facilities with exterior windows, if applicable, including management of environmental conditions (i.e., temperature and photoperiod control) and potential security risks.

8. Storage areas for flammable or hazardous agents and materials (e.g., disinfectants, cage-washing chemicals, pesticides, fuel).

I. Bioscience Research Building (BSRB)1. General arrangement of the animal facilities (conventional, clean/dirty corridor, etc.).The Biomedical Sciences Research Building (BSRB) is located across the street from the main CHS centralized vivarium. The vivarium is located in the basement level of BSRB, managed and serviced by DLAM. This vivarium designated for rodent housing. BSRB has 8 suites of dedicated mouse housing; each has 3 to 4 animal holding rooms and 1 to 2 procedure rooms. All suites are arranged along the main corridors – single corridor system 2. Physical relationship of the animal facilities to the research laboratories where animals may be used.

Research laboratories are located on the upper floors of BSRB. Animals from BSRB restricted access rodent breeding suites are also being transferred out to various buildings on campus. 3. Types of available animal housing spaces used, such as conventional, barrier, solation/quarantine, hazard containment (infectious, radioactive, chemical), “animal cubicles” or facilities specifically designed for housing certain species such as ponds, pastures, feedlots, etc.

BSRB is a designated SPF rodent facility. 5 suites are designated for restricted access mouse breeding colony, 2 suites are designated for ABSL2 immunocompromised rodent and 1 for conventional rodent housing.4. Finishes used throughout the animal facility for floors, walls, ceilings, doors, alleyways, gates, etc. (note any areas that are not easily sanitized and describe how these are maintained).

Floors - Animal rooms have seamless epoxy Stonhard floors. The flooring material extended 4 inches up the wall in most rooms to cover the wall-floor junction.Walls and Ceilings - All walls and ceilings are made of plaster and finished with epoxy paint.Doors – All doors are insulated metal doors, 42 inches wide by 84 inches high. Most doors

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have covered or tinted windows and some have no windows. The doors have push and kick plates.5. Engineering features (design, layout, special HVAC systems, noting exhaust air treatment, if applicable) used in hazardous agent containment.

Two designated ABSL2 suites have dedicated HVAC system. The HVAC systems serving the vivarium are single-duct, constant volume, with Hot Water Heating reheat coils. The Building Animation System monitors and controls each room’s supply and exhaust CFM, and regulates the temperature via Normally Closed reheat valves. The supply and exhaust zone boxes are tied to one controller allowing for accurate room pressurization control. 6. Security features, such as control of entry, perimeter fences, gates, entryways, cameras, guards; identify and describe exceptions for individual facilities or areas incorporating fewer or additional security features than the general features described.All of BSRB vivarium entrances are secured by card readers. All suites inside the vivarium are also equipped with security card readers. All animal holding rooms are secured by OMNI and key locks.7. Consideration for facilities with exterior windows, if applicable, including management of environmental conditions (i.e., temperature and photoperiod control) and potential security risks.

There is no exterior window in this facility. Each of the animal holding room is equipped with an environmental monitoring device (Sensoscientific Environmental Monitoring System). Temperature and humidity are monitored 24/7 with alarm notification sent via email/text messages to the vivarium manager on call. SensoScientific Company is working on light sensor capability to be implemented onto the existing monitoring devices. DLAM staffs are assigned to physically check automatic light timers in all animal holding rooms before 6:00am and after 6:00pm once monthly. 8. Storage areas for flammable or hazardous agents and materials (e.g., disinfectants, cage-washing chemicals, pesticides, fuel).BSRB has special chemical distribution system setup: Cage-washing chemical are stored in 200 gallons tank inside the designated chemical storage room on the floor above the vivarium where the building loading dock is located; the chemical is pumped directly into the cage-washing equipment in the B level vivarium. Small quantity of disinfectant are kept in 1-gallon containers in designated storage room in the vivarium.II. Brain Research Institute (BRI)1. General arrangement of the animal facilities (conventional, clean/dirty corridor, etc.).BRI is located within the CHS complex, west of the central Vivarium tower, near Neuropsychiatric Institute (NPI). There are 6 floors: 1, 2, 3, 4, 5 and 6, with 1 to 2 animal holding rooms, procedure rooms and-or storage rooms on each level. BRI vivarium is setup as vertical corridor with dedicated vivarium freight elevator.2. Physical relationship of the animal facilities to the research laboratories where animals may be used.

The animal rooms in BRI are at the west end of CHS corridor 3; various research labs occupied the CHS complex. 3. Types of available animal housing spaces used, such as conventional, barrier, solation/quarantine, hazard containment (infectious, radioactive, chemical), “animal cubicles”

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or facilities specifically designed for housing certain species such as ponds, pastures, feedlots, etc.

BRI facility is designated for conventional rodent housing. NHP are also housed in this facility. This vivarium is also hosting two ARC-approved “Study Areas”. 4. Finishes used throughout the animal facility for floors, walls, ceilings, doors, alleyways, gates, etc. (note any areas that are not easily sanitized and describe how these are maintained).

Floors - Animal rooms have seamless epoxy Stonhard floors. The flooring material extended 4 inches up the wall in most rooms to cover the wall-floor junction.Walls and Ceilings - All walls and ceilings are made of plaster and finished with epoxy paint.Doors - The metal doors are 44 inches wide by 84 inches high. The doors open into the animal rooms and are self-closing. Some doors have covered windows; some have no windows. They are equipped with locks and kept locked at all times. The doors have kick plates.5. Engineering features (design, layout, special HVAC systems, noting exhaust air treatment, if applicable) used in hazardous agent containment.

BRI facility has a dedicated HVAC system. Both supply and exhaust fans are constant-volume configuration; 100% exhaust. 6. Security features, such as control of entry, perimeter fences, gates, entryways, cameras, guards; identify and describe exceptions for individual facilities or areas incorporating fewer or additional security features than the general features described.BRI’s sensitive and high traffic areas on the 2nd,4th and 5th floor entry points are monitored by security surveillance cameras. Vivarium entry doors on all floors and BRI vivarium freight elevator are secured by card readers. Room doors have key-locks.7. Consideration for facilities with exterior windows, if applicable, including management of environmental conditions (i.e., temperature and photoperiod control) and potential security risks.

There is no exterior window in this facility. Each of the animal holding room is equipped with an environmental monitoring device (Sensoscientific Environmental Monitoring System). Temperature and humidity are monitored 24/7 with alarm notification sent via email/text messages to the vivarium manager on call. SensoScientific Company is working on light sensor capability to be implemented onto the existing monitoring devices. DLAM staffs are assigned to physically check automatic light timers in all animal holding rooms before 6:00am and after 6:00pm once monthly. 8. Storage areas for flammable or hazardous agents and materials (e.g., disinfectants, cage-washing chemicals, pesticides, fuel).

Small quantity of disinfectant are kept in 1-gallon containers in designated storage room.

III. Center for Health Science (CHS)1. General arrangement of the animal facilities (conventional, clean/dirty corridor, etc.).The Center for the Health Sciences (CHS) Vivarium is the main centralized vivarium in an 8-floors tower including underground levels BV and AV. Most animals are housed and managed by DLAM (Radiation Oncology, an independent vivarium is located on the 6thfloor of this tower) along with procedure and office space on the B, 1st, 2nd, 3rd, 4th, 5th, 6th and 8th levels (AV level is designated for staff offices, conference and staff training rooms). This

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vivarium has a single corridor system.

2. Physical relationship of the animal facilities to the research laboratories where animals may be used.The research labs serviced by this vivarium tower are located at various location in CHS complex, as well as multiple buildings on campus.3. Types of available animal housing spaces used, such as conventional, barrier, solation/quarantine, hazard containment (infectious, radioactive, chemical), “animal cubicles” or facilities specifically designed for housing certain species such as ponds, pastures, feedlots, etc.

CHS vivarium tower housed multiple species of animals, primarily rodents:

BV - This facility is managed and serviced by DLAM and houses mainly mice. There is a designated USDA covered species recovery rooms on this floor.

AV – This floor has DLAM staff offices, staff training and conference rooms.

1V - Contains DLAM managed housing rooms for mice, rats, chinchillas, gerbils, lizards, Guinea pigs, rabbits, and geckos. There are 2 designated ABSL2 rodent rooms located on this floor. NHP (new arrival) quarantine rooms are located on this floor. DLAM vivarium dedicated and restricted receiving loading dock, Cage washing facility, central (animal and supply) receiving and storeroom, break room and offices are located on this floor.

2V - Contains DLAM managed housing rooms for rats and mice. Central surgery facility for rodents and USDA covered species are located on this floor.

3V – is the centralized ABSL2/2+ hazardous containment vivarium, designated for housing of rodents and USDA covered species; managed by DLAM. The DLAM ART Lab is also located on this floor. There is a PI-managed (Study Area) frog room located on this floor.

4V - This facility contained a Gnotobiotic facility and a SPF barrier mouse breeding colony managed by DLAM. There’s a cage washing and sterilizers machines dedicated to servicing this floor. Access to this facility is restricted.

5V - This facility has DLAM Clinical Diagnostic and Molecular Diagnostic Labs, a Surgical Training Room, and a Necropsy room, all managed by DLAM. Frogs, mice, rats, and sea lampreys are housed on this floor and managed by DLAM. There is also a researcher- managed (Study area) Cardiovascular Physiology and Telemetry lab on this floor within the vivarium area.

6V - This floor contains rat rooms and pharmacy managed by DLAM. There are three PI managed research labs (Study Areas) on this level within the vivarium area. A Defined Flora barrier facility equipped with cage-washing and autoclaving facility managed by the Department of Radiation Oncology is also located on this floor.

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8V - This facility houses swine and canines. Additionally, there is a cage washing room containing a cage-rack washer, a feed storage refrigerator, a locker room for animal technicians and a small veterinary clinic (K9 Clinic).

4. Finishes used throughout the animal facility for floors, walls, ceilings, doors, alleyways, gates, etc. (note any areas that are not easily sanitized and describe how these are maintained).

Floors - Animal rooms have seamless epoxy Stonhard floors. The flooring material extended 4 inches up the wall in most rooms to cover the wall-floor junction. There are multiple rooms with original tile flooring.Walls and Ceilings - All walls and ceilings are made of plaster and finished with epoxy paint.Doors - The metal doors are 42 inches wide by 84 inches high. The doors open into the animal rooms and are self-closing. Some doors have covered windows; some have no windows. They are equipped with key-locks and kept locked at all times.5. Engineering features (design, layout, special HVAC systems, noting exhaust air treatment, if applicable) used in hazardous agent containment.CHS vivarium facility has a dedicated HVAC system. The ABSL2/2+ facility on 3V has dedicated HVAC system. The main HVAC system serving the vivarium is double-duct with Hot Water Heating reheat coils. Both supply and exhaust fans are constant-volume configuration; all with 100% exhaust.6. Security features, such as control of entry, perimeter fences, gates, entryways, cameras, guards; identify and describe exceptions for individual facilities or areas incorporating fewer or additional security features than the general features described.All of CHS vivarium tower entrances and sensitive areas entry points are monitored by security surveillance cameras. Vivarium entry doors on all floors including the vivarium freight elevator are secured by card readers. Room doors have key-locks.7. Consideration for facilities with exterior windows, if applicable, including management of environmental conditions (i.e., temperature and photoperiod control) and potential security risks.There is no exterior window in this facility. Each of the animal holding room is equipped with an environmental monitoring device (Sensoscientific Environmental Monitoring System). Temperature and humidity are monitored 24/7 with alarm notification sent via email/text messages to the vivarium manager on call. SensoScientific Company is working on light sensor capability to be implemented onto the existing monitoring devices. DLAM staffs are assigned to physically check automatic light timers in all animal holding rooms before 6:00am and after 6:00pm once monthly.8. Storage areas for flammable or hazardous agents and materials (e.g., disinfectants, cage-washing chemicals, pesticides, fuel).

IV. California NanoSystems Institute (CNSI)1. General arrangement of the animal facilities (conventional, clean/dirty corridor, etc.).CNSI vivarium and Crump imagining center is located on the 2nd floor of CNSI building; North of the central CHS vivarium tower. This vivarium is serviced by DLAM.2. Physical relationship of the animal facilities to the research laboratories where animals may be used.

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Research labs and imaging suite is located adjacent to the vivarium3. Types of available animal housing spaces used, such as conventional, barrier, isolation/quarantine, hazard containment (infectious, radioactive, chemical), “animal cubicles” or facilities specifically designed for housing certain species such as ponds, pastures, feedlots, etc.

CNSI housed SPF rodents. There is a single ABSL2 animal housing room, a procedure room and a ‘hot’ animal holding room where animals are held during radioactive decay following imaging. 4. Finishes used throughout the animal facility for floors, walls, ceilings, doors, alleyways, gates, etc. (note any areas that are not easily sanitized and describe how these are maintained).

Floors - Animal rooms have seamless epoxy Stonehard floors. The flooring material extended 4 inches up the wall in most rooms to cover the wall-floor junction.Walls and Ceilings - All walls and ceilings are made of plaster and finished with epoxy paint.Doors - The metal doors are 44 inches wide by 84 inches high. The doors open into the animal rooms and are self-closing. Some doors have covered windows; some have no windows. They are equipped with locks and kept locked at all times. The doors have kick plates.5. Engineering features (design, layout, special HVAC systems, noting exhaust air treatment, if applicable) used in hazardous agent containment.

CNSI’s HVAC system serving the vivarium is dedicated single-duct, constant volume, with Hot Water Heating reheat coils. The Building Animation System monitors and controls room’s supply and exhaust CFM, and regulates the temperature via Normally Closed reheat valves. The supply and exhaust zone boxes are tied to one controller allowing for accurate room pressurization control.5. Security features, such as control of entry, perimeter fences, gates, entryways, cameras, guards; identify and describe exceptions for individual facilities or areas incorporating fewer or additional security features than the general features described.

CNSI vivarium entrances are secured by card readers. Room doors inside the vivarium have key-locks.7. Consideration for facilities with exterior windows, if applicable, including management of environmental conditions (i.e., temperature and photoperiod control) and potential security risks.

There is no exterior window in this facility. Each of the animal holding room is equipped with an environmental monitoring device (Sensoscientific Environmental Monitoring System). Temperature and humidity are monitored 24/7 with alarm notification sent via email/text messages to the vivarium manager on call. SensoScientific Company is working on light sensor capability to be implemented onto the existing monitoring devices. DLAM staffs are assigned to physically check automatic light timers in all animal holding rooms before 6:00am and after 6:00pm once monthly. 8. Storage areas for flammable or hazardous agents and materials (e.g., disinfectants, cage-washing chemicals, pesticides, fuel).

V. Franz Hall

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1. General arrangement of the animal facilities (conventional, clean/dirty corridor, etc.).Franz Hall vivarium supports The Department of Psychology, located in the central UCLA campus (north of central CHS vivarium tower) on 2 floors B and C below ground level. All rooms are arranged along the main corridors – single corridor system 2. Physical relationship of the animal facilities to the research laboratories where animals may be used.

Research labs and the vivarium are located on the same level and share the same corridors3. Types of available animal housing spaces used, such as conventional, barrier, solation/quarantine, hazard containment (infectious, radioactive, chemical), “animal cubicles” or facilities specifically designed for housing certain species such as ponds, pastures, feedlots, etc.

Franz Hall vivarium housed primarily conventional rat and mice; there are also pigeons housed in this building4. Finishes used throughout the animal facility for floors, walls, ceilings, doors, alleyways, gates, etc. (note any areas that are not easily sanitized and describe how these are maintained).

Floors - Animal rooms have seamless epoxy floors. The flooring material extended 4 inches up the wall in most rooms to cover the wall-floor junction.Walls and Ceilings - All walls and ceilings are made of plaster and finished with epoxy paint.Doors - The metal doors are 42 inches wide by 84 inches high. The doors open into the animal rooms and are self-closing. Some doors have covered windows; some have no windows. They are equipped with locks and kept locked at all times. 5. Engineering features (design, layout, special HVAC systems, noting exhaust air treatment, if applicable) used in hazardous agent containment.

Franz Hall vivarium main HVAC system is double-duct configuration. Both supply and exhaust fans are constant-volume configuration; all with 100% exhaust.6. Security features, such as control of entry, perimeter fences, gates, entryways, cameras, guards; identify and describe exceptions for individual facilities or areas incorporating fewer or additional security features than the general features described.Franz Hall vivarium entrances and sensitive areas entry points are monitored by security surveillance cameras. Vivarium entry doors on all floors including the building freight and regular elevators accessing the vivarium floors are secured by card readers. Room doors inside the vivarium have key-locks.7. Consideration for facilities with exterior windows, if applicable, including management of environmental conditions (i.e., temperature and photoperiod control) and potential security risks.

There is no exterior window in this facility. Each of the animal holding room is equipped with an environmental monitoring device (Sensoscientific Environmental Monitoring System). Temperature and humidity are monitored 24/7 with alarm notification sent via email/text messages to the vivarium manager on call. SensoScientific Company is working on light sensor capability to be implemented onto the existing monitoring devices. DLAM staffs are assigned to physically check automatic light timers in all animal holding rooms before 6:00am and after 6:00pm once monthly. 8. Storage areas for flammable or hazardous agents and materials (e.g., disinfectants,

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cage-washing chemicals, pesticides, fuel).Cage-washing chemical are kept in 30-gallon barrels inside the cage-washing room. Small quantity of disinfectant are kept in 1-gallon containers in designated storage room.

VI. Gonda Genetics Institute1. General arrangement of the animal facilities (conventional, clean/dirty corridor, etc.).Gonda vivarium is located on the B level of Gonda building in South campus across the street from CHS central vivarium tower. This facility is a dual clean-soiled corridor with animal holding rooms on either side. Each animal room has 2 doors, one entry from clean corridor and one exit to soiled corridor. 2. Physical relationship of the animal facilities to the research laboratories where animals may be used.

Research labs located on the upper floors of Gonda buildings3. Types of available animal housing spaces used, such as conventional, barrier, solation/quarantine, hazard containment (infectious, radioactive, chemical), “animal cubicles” or facilities specifically designed for housing certain species such as ponds, pastures, feedlots, etc.

Gonda vivarium is designated for SPF mouse housing. 4. Finishes used throughout the animal facility for floors, walls, ceilings, doors, alleyways, gates, etc. (note any areas that are not easily sanitized and describe how these are maintained).

Floors - Animal rooms have seamless epoxy floors. The flooring material extended 4 inches up the wall in most rooms to cover the wall-floor junction.Walls and Ceilings - All walls and ceilings are made of plaster and finished with epoxy paint.Doors - The metal doors are 42 inches wide by 84 inches high; there are 2 doors for each animal holding rooms. The doors open into the animal rooms and are self-closing. Some doors have covered windows; some have no windows. They are equipped with locks and kept locked at all times.5. Engineering features (design, layout, special HVAC systems, noting exhaust air treatment, if applicable) used in hazardous agent containment.

Gonda vivarium has a dedicated system serving the B level vivarium; setup with HEPA filters on the supply fans. The system is single-duct, constant volume. Each vivarium room is equipped with stand-alone controllers. The room temperature is controlled by modulating the Normally Closed reheat valve whereas the supply and exhaust volume dampers are controlled via digital velocity sensors; all with 100% exhaust.7. Security features, such as control of entry, perimeter fences, gates, entryways, cameras, guards; identify and describe exceptions for individual facilities or areas incorporating fewer or additional security features than the general features described.

Gonda vivarium’s sensitive areas and entry points are monitored by security surveillance cameras. Vivarium entry doors are secured by card readers. Room doors inside the vivarium have OMNI and key-locks.7. Consideration for facilities with exterior windows, if applicable, including management of environmental conditions (i.e., temperature and photoperiod control) and potential security risks.

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There is no exterior window in this facility. Each of the animal holding room is equipped with an environmental monitoring device (Sensoscientific Environmental Monitoring System). Temperature and humidity are monitored 24/7 with alarm notification sent via email/text messages to the vivarium manager on call. SensoScientific Company is working on light sensor capability to be implemented onto the existing monitoring devices. DLAM staffs are assigned to physically check automatic light timers in all animal holding rooms before 6:00am and after 6:00pm once monthly. 8. Storage areas for flammable or hazardous agents and materials (e.g., disinfectants, cage-washing chemicals, pesticides, fuel).Cage-washing chemical are kept in 30-gallon barrels inside the cage-washing room. Small quantity of disinfectant are kept in 1-gallon containers in designated storage room.

VII. Terasaki Life Science Building (TLSB)1. General arrangement of the animal facilities (conventional, clean/dirty corridor, etc.).TLSB vivarium is located on the B level, in south campus, East of the main CHS vivarium tower. There are 2 suites with 8 animal holding and 8 procedure rooms nested inside the SPF mouse barrier, along with a rodent return room inside a research lab suites outside of the barrier are managed and serviced by DLAM. All suites and rooms are arranged along the main single corridors system.2. Physical relationship of the animal facilities to the research laboratories where animals may be used.

Research labs are located on the upper floors and outside of the B level of TLSB building. 3. Types of available animal housing spaces used, such as conventional, barrier, solation/quarantine, hazard containment (infectious, radioactive, chemical), “animal cubicles” or facilities specifically designed for housing certain species such as ponds, pastures, feedlots, etc.

TLSB housed SPF rodents. There are also finch-birds housed in this vivarium.4. Finishes used throughout the animal facility for floors, walls, ceilings, doors, alleyways, gates, etc. (note any areas that are not easily sanitized and describe how these are maintained).Floors - Animal rooms have seamless epoxy Stonhard floors. The flooring material extended 4 inches up the wall in most rooms to cover the wall-floor junction.Walls and Ceilings - All walls and ceilings are made of plaster and finished with epoxy paint.Doors - The metal doors are 42 inches wide by 84 inches high. The doors open into the animal rooms and are self-closing. Some doors have covered windows; some have no windows. They are equipped with key-locks. The doors have push and kick plates.5. Engineering features (design, layout, special HVAC systems, noting exhaust air treatment, if applicable) used in hazardous agent containment.

The main HVAC system serving the vivarium is dedicated, a single-duct, constant volume, with Hot Water Heating reheat coils. Both supply and exhaust fans are constant-volume configuration; all with 100% exhaust.6. Security features, such as control of entry, perimeter fences, gates, entryways, cameras, guards; identify and describe exceptions for individual facilities or areas incorporating fewer

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or additional security features than the general features described.TLSB vivarium entry doors and suites doors are secured by card readers. Room doors

inside the vivarium have key-locks.7. Consideration for facilities with exterior windows, if applicable, including management of environmental conditions (i.e., temperature and photoperiod control) and potential security risks.

There is no exterior window in this facility. Each of the animal holding room is equipped with an environmental monitoring device (Sensoscientific Environmental Monitoring System). Temperature and humidity are monitored 24/7 with alarm notification sent via email/text messages to the vivarium manager on call. SensoScientific Company is working on light sensor capability to be implemented onto the existing monitoring devices. DLAM staffs are assigned to physically check automatic light timers in all animal holding rooms before 6:00am and after 6:00pm once monthly. 8. Storage areas for flammable or hazardous agents and materials (e.g., disinfectants, cage-washing chemicals, pesticides, fuel).Cage-washing chemical are kept in 30-gallon barrels inside the cage-washing room. Small quantity of disinfectant are kept in 1-gallon containers in designated storage room.

VIII. MacDonald Research Lab (MRL)1. General arrangement of the animal facilities (conventional, clean/dirty corridor, etc.).MRL is located north of CHS, across the street from the main CHS vivarium tower. This facility is managed and serviced by DLAM. The general arrangement of this facility is a dual clean-soiled corridor with animal holding rooms on either side. Each animal room has 2 doors, one entry from clean corridor and one exit to soiled corridor.2. Physical relationship of the animal facilities to the research laboratories where animals may be used.

Research laboratories are located on the upper floors throughout MRL building.3. Types of available animal housing spaces used, such as conventional, barrier, solation/quarantine, hazard containment (infectious, radioactive, chemical), “animal cubicles” or facilities specifically designed for housing certain species such as ponds, pastures, feedlots, etc.

MRL is a SPF mouse facility.4. Finishes used throughout the animal facility for floors, walls, ceilings, doors, alleyways, gates, etc. (note any areas that are not easily sanitized and describe how these are maintained).Floors - Animal rooms have seamless epoxy Stonhard floors. The flooring material extended 4 inches up the wall in most rooms to cover the wall-floor junction.Walls and Ceilings - All walls and ceilings are made of plaster and finished with epoxy paint.Doors - The metal doors are 42 inches wide by 84 inches high. The doors open into the animal rooms and are self-closing. Some doors have covered windows; some have no windows. They are equipped with key-locks. The doors have push and kick plates.5. Engineering features (design, layout, special HVAC systems, noting exhaust air treatment, if applicable) used in hazardous agent containment.

MRL vivarium has a dedicated HVAC system serving the B level vivarium. The

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system is single-duct, constant volume. Each vivarium room is equipped with stand-alone controllers. The room temperature is controlled by modulating the Normally Closed reheat valve whereas the supply and exhaust volume dampers are controlled via digital velocity sensors; all with 100% exhaust.6. Security features, such as control of entry, perimeter fences, gates, entryways, cameras, guards; identify and describe exceptions for individual facilities or areas incorporating fewer or additional security features than the general features described.

All of MRL vivarium entrances and sensitive areas entry points are monitored by security surveillance cameras. Vivarium entry doors are secured by card readers. Room doors inside the vivarium have key-locks.7. Consideration for facilities with exterior windows, if applicable, including management of environmental conditions (i.e., temperature and photoperiod control) and potential security risks.

There is no exterior window in this facility. Each of the animal holding room is equipped with an environmental monitoring device (Sensoscientific Environmental Monitoring System). Temperature and humidity are monitored 24/7 with alarm notification sent via email/text messages to the vivarium manager on call. SensoScientific Company is working on light sensor capability to be implemented onto the existing monitoring devices. DLAM staffs are assigned to physically check automatic light timers in all animal holding rooms before 6:00am and after 6:00pm once monthly. 8. Storage areas for flammable or hazardous agents and materials (e.g., disinfectants, cage-washing chemicals, pesticides, fuel).Cage-washing chemical are kept in 30-gallon barrels inside the cage-washing room. Small quantity of disinfectant are kept in 1-gallon containers in designated storage room.

IX. Neuroscience Research Building (NRB)1. General arrangement of the animal facilities (conventional, clean/dirty corridor, etc.).The Neuroscience Research Building is located across the street from CHS vivarium tower. Animal holding and procedure rooms occupy 4 floors within the secured vivarium and are managed/serviced by DLAM. This vivarium has a suite arrangement, each with its own procedure room. The NHP area includes holding, surgical, procedural and testing rooms adjacent to the investigator’s laboratory.

2. Physical relationship of the animal facilities to the research laboratories where animals may be used.

Research laboratories are located on the upper floors throughout NRB3. Types of available animal housing spaces used, such as conventional, barrier, solation/quarantine, hazard containment (infectious, radioactive, chemical), “animal cubicles” or facilities specifically designed for housing certain species such as ponds, pastures, feedlots, etc.

NRB is designated for SPF rodents housing, primarily mice. NHP are housed on separate floor in this building.4. Finishes used throughout the animal facility for floors, walls, ceilings, doors, alleyways, gates, etc. (note any areas that are not easily sanitized and describe how these are

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maintained).Floors - Animal rooms have seamless epoxy (Stonhard) floors. The flooring material extended 4 inches up the wall in most rooms to cover the wall-floor junction.Walls and Ceilings - All walls and ceilings are made of plaster and finished with epoxy paint.Doors - The metal doors are 42 inches wide by 84 inches high. The doors open into the animal rooms and are self-closing. Some doors have covered windows; some have no windows. They are equipped with key-locks. The doors have push and kick plates.5. Engineering features (design, layout, special HVAC systems, noting exhaust air treatment, if applicable) used in hazardous agent containment.

The HVAC systems serving the vivarium are single-duct, constant volume, with Hot Water Heating reheat coils. The Building Animation System monitors and controls each room’s supply and exhaust CFM, and regulates the temperature via Normally Closed reheat valves. The supply and exhaust zone boxes are tied to one controller allowing for accurate room pressurization control.6. Security features, such as control of entry, perimeter fences, gates, entryways, cameras, guards; identify and describe exceptions for individual facilities or areas incorporating fewer or additional security features than the general features described.

All of NRB vivarium entrances and sensitive areas entry points are monitored by security surveillance cameras. All vivarium entry doors on all floors including the vivarium and building’s freight elevators are secured by card readers. Room doors inside the vivarium have OMNI and key-locks.7. Consideration for facilities with exterior windows, if applicable, including management of environmental conditions (i.e., temperature and photoperiod control) and potential security risks.

There is no exterior window in this facility. Each of the animal holding room is equipped with an environmental monitoring device (Sensoscientific Environmental Monitoring System). Temperature and humidity are monitored 24/7 with alarm notification sent via email/text messages to the vivarium manager on call. SensoScientific Company is working on light sensor capability to be implemented onto the existing monitoring devices. DLAM staffs are assigned to physically check automatic light timers in all animal holding rooms before 6:00am and after 6:00pm once monthly. 8. Storage areas for flammable or hazardous agents and materials (e.g., disinfectants, cage-washing chemicals, pesticides, fuel).Cage-washing chemical are kept in 30-gallon barrels inside the cage-washing room. Small quantity of disinfectant are kept in 1-gallon containers in designated storage room.

X. Public Health (PH)1. General arrangement of the animal facilities (conventional, clean/dirty corridor, etc.).Public Health is located adjacent to the CHS Vivarium; connected to CHS BV level (using same corridor) and consisting of one floor of mouse holding rooms managed by DLAM.2. Physical relationship of the animal facilities to the research laboratories where animals may be used.

The research labs are located at various location in CHS complex, as well as multiple other research buildings on campus.3. Types of available animal housing spaces used, such as conventional, barrier,

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solation/quarantine, hazard containment (infectious, radioactive, chemical), “animal cubicles” or facilities specifically designed for housing certain species such as ponds, pastures, feedlots, etc.

PH vivarium is designated for housing SPF mice.4. Finishes used throughout the animal facility for floors, walls, ceilings, doors, alleyways, gates, etc. (note any areas that are not easily sanitized and describe how these are maintained).Floors - Animal rooms have seamless epoxy Stonhard floors. The flooring material extended 4 inches up the wall in most rooms to cover the wall-floor junction.Walls and Ceilings - All walls and ceilings are made of plaster and finished with epoxy paint.Doors - The metal doors are 42 inches wide by 84 inches high. The doors open into the animal rooms and are self-closing. Some doors have covered windows; some have no windows. They are equipped with key-locks. The doors have push and kick plates.5. Engineering features (design, layout, special HVAC systems, noting exhaust air treatment, if applicable) used in hazardous agent containment.

Public Health vivarium has a dedicated HVAC system. Both supply and exhaust fans are constant-volume configuration; 100% exhaust.6. Security features, such as control of entry, perimeter fences, gates, entryways, cameras, guards; identify and describe exceptions for individual facilities or areas incorporating fewer or additional security features than the general features described.

All of Public Health vivarium entrances are monitored by security surveillance cameras. Vivarium entry doors are secured by card readers. All room doors inside the vivarium have key-locks.7. Consideration for facilities with exterior windows, if applicable, including management of environmental conditions (i.e., temperature and photoperiod control) and potential security risks.

There is no exterior window in this facility. Each of the animal holding room is equipped with an environmental monitoring device (Sensoscientific Environmental Monitoring System). Temperature and humidity are monitored 24/7 with alarm notification sent via email/text messages to the vivarium manager on call. SensoScientific Company is working on light sensor capability to be implemented onto the existing monitoring devices. DLAM staffs are assigned to physically check automatic light timers in all animal holding rooms before 6:00am and after 6:00pm once monthly. 8. Storage areas for flammable or hazardous agents and materials (e.g., disinfectants, cage-washing chemicals, pesticides, fuel).Cage-washing chemical are kept in 30-gallon barrels inside the cage-washing room. Small quantity of disinfectant are kept in 1-gallon containers in designated storage room.

XI. Rehab Center* No Animal – Insufficient HVAC system - Equipment Storage Only *1. General arrangement of the animal facilities (conventional, clean/dirty corridor, etc.).Rehab Center is located on the Southwest corner of UCLA central campus; approximately one miles from the main CHS vivarium tower and across the street from Warren Hall vivarium.2. Physical relationship of the animal facilities to the research laboratories where animals may be used.

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NA3. Types of available animal housing spaces used, such as conventional, barrier, solation/quarantine, hazard containment (infectious, radioactive, chemical), “animal cubicles” or facilities specifically designed for housing certain species such as ponds, pastures, feedlots, etc.

NA4. Finishes used throughout the animal facility for floors, walls, ceilings, doors, alleyways, gates, etc. (note any areas that are not easily sanitized and describe how these are maintained).

NA5. Engineering features (design, layout, special HVAC systems, noting exhaust air treatment, if applicable) used in hazardous agent containment.

NA6. Security features, such as control of entry, perimeter fences, gates, entryways, cameras, guards; identify and describe exceptions for individual facilities or areas incorporating fewer or additional security features than the general features described.

Rehab Center’s room doors have OMNI and key-locks.7. Consideration for facilities with exterior windows, if applicable, including management of environmental conditions (i.e., temperature and photoperiod control) and potential security risks.

NA8. Storage areas for flammable or hazardous agents and materials (e.g., disinfectants, cage-washing chemicals, pesticides, fuel).

NA

XII. Slichter Hall* No Animals in vivarium area – Equipment Storage Only *1. General arrangement of the animal facilities (conventional, clean/dirty corridor, etc.).

Slichter Hall is located in Central campus, adjacent to Franz Hall vivarium, North of CHS vivarium tower.2. Physical relationship of the animal facilities to the research laboratories where animals may be used.

NA3. Types of available animal housing spaces used, such as conventional, barrier, solation/quarantine, hazard containment (infectious, radioactive, chemical), “animal cubicles” or facilities specifically designed for housing certain species such as ponds, pastures, feedlots, etc.

NA4. Finishes used throughout the animal facility for floors, walls, ceilings, doors, alleyways, gates, etc. (note any areas that are not easily sanitized and describe how these are maintained).

NA5. Engineering features (design, layout, special HVAC systems, noting exhaust air treatment, if applicable) used in hazardous agent containment.

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NA6. Security features, such as control of entry, perimeter fences, gates, entryways, cameras, guards; identify and describe exceptions for individual facilities or areas incorporating fewer or additional security features than the general features described.

Slichter Hall facility’s room doors have key-locks.

XIII. Warren Hall1. General arrangement of the animal facilities (conventional, clean/dirty corridor, etc.).Warren Hall Vivarium is designated for rodent housing, nested on the 2nd floor, north-western wing of Warren Hall building, which is located on the Southwest corner of UCLA central campus; approximately 1 miles from the main CHS vivarium tower. Animal holding, procedure, cage wash and storage rooms are arranged along the main corridors – single corridor system.2. Physical relationship of the animal facilities to the research laboratories where animals may be used.

Laboratories are located throughout Warren Hall buildings and adjacent Hillbloom research building.3. Types of available animal housing spaces used, such as conventional, barrier, solation/quarantine, hazard containment (infectious, radioactive, chemical), “animal cubicles” or facilities specifically designed for housing certain species such as ponds, pastures, feedlots, etc.

This vivarium housed conventional rodent.4. Finishes used throughout the animal facility for floors, walls, ceilings, doors, alleyways, gates, etc. (note any areas that are not easily sanitized and describe how these are maintained).Floors - Animal rooms have seamless epoxy floors. The flooring material extended 4 inches up the wall in most rooms to cover the wall-floor junction.Walls and Ceilings - All walls and ceilings are made of plaster and finished with epoxy paint.Doors - The metal doors are 42 inches wide by 84 inches high. The doors open into the animal rooms and are self-closing. Some doors have covered windows; some have no windows. They are equipped with key-locks. The doors have push and kick plates.5. Engineering features (design, layout, special HVAC systems, noting exhaust air treatment, if applicable) used in hazardous agent containment.

Warren Hall has a dedicated HVAC system. Both supply and exhaust fans are constant-volume configuration; 100% exhaust.6. Security features, such as control of entry, perimeter fences, gates, entryways, cameras, guards; identify and describe exceptions for individual facilities or areas incorporating fewer or additional security features than the general features described.

Warren Hall vivarium entrances and main corridor are monitored by security surveillance cameras. Vivarium entry doors are secured by card readers. Room doors inside the vivarium have key-locks.7. Consideration for facilities with exterior windows, if applicable, including management of environmental conditions (i.e., temperature and photoperiod control) and potential security risks.

There is no exterior window in this facility. Each of the animal holding room is

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equipped with an environmental monitoring device (Sensoscientific Environmental Monitoring System). Temperature and humidity are monitored 24/7 with alarm notification sent via email/text messages to the vivarium manager on call. SensoScientific Company is working on light sensor capability to be implemented onto the existing monitoring devices. DLAM staffs are assigned to physically check automatic light timers in all animal holding rooms before 6:00am and after 6:00pm once monthly.9. Storage areas for flammable or hazardous agents and materials (e.g., disinfectants, cage-washing chemicals, pesticides, fuel).Cage-washing chemical are kept in 30-gallon barrels inside the cage-washing room. Small quantity of disinfectant are kept in 1-gallon containers in designated storage room.

XIV. Doheny Eye Institute (DEI)1. General arrangement of the animal facilities (conventional, clean/dirty corridor, etc.).Doheny Eye Institute is located on the University of Southern California (USC) campus; approximately 20 miles East of UCLA campus. The vivarium is located on the second floor of the building; serviced by DLAM.2. Physical relationship of the animal facilities to the research laboratories where animals may be used. The research labs are located at various locations on the adjacent corridors and upper floors.3. Types of available animal housing spaces used, such as conventional, barrier, solation/quarantine, hazard containment (infectious, radioactive, chemical), “animal cubicles” or facilities specifically designed for housing certain species such as ponds, pastures, feedlots, etc. DEI vivarium is designated for SPF rodents housing. There are 2 rodent holding rooms; one is approved for ABSL2 studies (currently empty). There are storage and procedure rooms nested inside the vivarium.4. Finishes used throughout the animal facility for floors, walls, ceilings, doors, alleyways, gates, etc. (note any areas that are not easily sanitized and describe how these are maintained).Floors - Animal rooms have vinyl tiles with plastic floor molding extended 3 inches up to cover the wall-floor junction.Walls and Ceilings - All walls and ceilings are made of plaster and finished with epoxy paint.Doors - The metal doors are 44 inches wide by 84 inches high. The doors open into the animal rooms and are self-closing. Animal room doors have no windows. They are equipped with key-locks and are kept locked at all times 5. Engineering features (design, layout, special HVAC systems, noting exhaust air treatment, if applicable) used in hazardous agent containment. DEI vivarium has a dedicated HVAC system with 100% exhaust.6. Security features, such as control of entry, perimeter fences, gates, entryways, cameras, guards; identify and describe exceptions for individual facilities or areas incorporating fewer or additional security features than the general features described. There are security cameras located at the public entry point on the second floor and within the vivarium. The vivarium entry door is secured by a card reader and animal holding room doors have key-locks.

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7. Consideration for facilities with exterior windows, if applicable, including management of environmental conditions (i.e., temperature and photoperiod control) and potential security risks. There are no exterior windows in this facility. Each of the animal holding rooms is equipped with an environmental monitoring device (Sensoscientific Environmental Monitoring System). Temperature and humidity are monitored 24/7 with alarm notification sent via email/text messages to the vivarium manager on call. The animal holding room is also equipped with a portable humidifier in case of low humidity. 8. Storage areas for flammable or hazardous agents and materials (e.g., disinfectants, cage-washing chemicals, pesticides, fuel).Small quantity of disinfectant is kept in 1-gallon containers in designated storage room.

C. Satellite Animal Housing FacilitiesIn addition to the Appendices summarizing Heating, Ventilation, and Air-Conditioning (Appendix 11) and Lighting Systems (Appendix 16), summarize animal housing areas that are not centrally-managed or maintained in (Appendix 17), “Satellite Animal Housing Areas.”

1. Describe the criteria used to determine/define a “Satellite Animal Housing Area,” which may include remote housing facilities or laboratories temporarily or consistently housing animals.

UCLA uses “Study Area” instead of “Satellite Animal Housing Area.” AWA 9 CFR 1, section 1.1.(5) defines “Study Area” as any building room, area, enclosure, or other containment outside of a core facility or centrally designated or managed area in which animals are housed for more than 12 hours.

The ARC Policy on Maintaining Animals in Study Areas defines a Study Area as follows:

‘Any investigator-managed building, room, area, enclosure, or other containment site in which USDA-regulated animal species [1] are housed for periods longer than 12 hours, or in which non-USDA-regulated animal species [2] are housed for periods longer than 24 hours.’

2. Describe the process used by the IACUC/OB to authorize, provide oversight of, and ensure compliance with Guide standards for the housing of animals outside of centrally-maintained facilities. Include a description of Attending Veterinarian access and physical security.

The ARC approves the use of study areas on a case-by-case basis. Animals may be housed in study areas provided (from ARC policy): ‘Scientific justification for this arrangement is approved by the ARC. Please note that

convenience is not considered acceptable justification for use of a study area. In rare cases, certain species may be routinely housed outside of the DLAM-managed vivarium when DLAM facilities are inadequate for their appropriate housing; as with

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other study areas, the ARC must review and approve these requests. Please note that the ARC may rescind approval of any study area at such time as suitable vivarium housing becomes available.

The study area is inspected and certified by the ARC at least once every six months. ARC certification of a study area is valid for a 6-month period after the date of

inspection with the condition that acceptable standards are maintained. The DLAM Animal Health Technician (AHT) responsible for monitoring study areas

[3] is notified when animals are brought to and removed from a study area in order to facilitate the identification of active areas which require oversight by the ARC and DLAM.

A Standard Operating Procedure (SOP) for management of the study area is developed by the investigator and approved by the ARC. The SOP includes information on husbandry requirements, daily monitoring of the animals, provision of food and water, bedding and cage changing, pest control, record keeping, Occ. Health, etc.

Daily study area logs are maintained for periods when animals are present and retained for inspection by the ARC and/or DLAM staff for at least 6 months. (see Section IV.C.1).

Ventilation in the study area is adequate as measured by DLAM or Facilities Management (see Sections IV.A.4 and IV.C.3).

The Campus Veterinarian or designee is given access (i.e., a key or combination) to the study area for evaluation of animal health and well-being (see Section V). Note: 24-hour access to the study area must be provided.’

The aforementioned ARC Policy on Maintaining Animals in Study Areas includes detailed guidelines for animal environment, housing, and management in PI-managed housing areas. These locations are inspected semi-annually by the ARC. Also, as stated in the Policy:

‘The Campus Veterinarian must be given access (i.e., a key or combination) to the study area in order to ensure the provision of adequate veterinary care in accordance with federal requirements. Specifically, the USDA AWARs §2.33(a)(2) mandates that "each research facility shall assure that the attending veterinarian has appropriate authority to ensure the provision of adequate veterinary care and to oversee the adequacy of other aspects of animal care and use." Furthermore, the Guide (p. 14) states that "the attending veterinarian (AV) is responsible for the health and well-being of all laboratory animals used at the institution," and that "the institution must provide the AV with sufficient authority, including access to animals, and resources to manage the program of veterinary care." Similarly, the Association for Assessment and Accreditation of Laboratory Animal Care (AAALAC) International requires that "the attending veterinarian must have access to the institution's animals used in teaching and research." As described in the ARC Policy Authority of the Attending Veterinarian, “The attending veterinarian must have unrestricted access to all areas where animals are used or housed (including the vivarium, research laboratories, and research study areas).” Such access must be available 24-hours/day, 7 days/week.’

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DLAM employs an animal health technician dedicated to the oversight of all study areas. This staff person visits each study area on a weekly basis and checks on animal health and, when necessary, submits animal health reports to a DLAM veterinarian. This person also monitors and consults with ARC staff on compliance related issues such as the maintenance of daily room logs and other required animal care logs, housekeeping and other issues. The technician keeps a log of the visits (any comments or findings) in an Excel file to allow for regulatory review by the ARC at any time, and will be available for review at the time of the site visit, upon request.

D. Emergency Power and Life Support Systems Note: Complete a Heating, Ventilation, and Air-Conditioning (HVAC) Summary (Appendix 11) and Lighting Summary (Appendix 16) for each Location described in the Summary of Animal Housing and Support Sites (Appendix 2).

1. Power [Guide, p. 141]For each Location, Centralized Animal Facility, and Satellite Housing Facility, provide a brief description of the following: Availability of emergency power and if so, what electrical services and equipment

are maintained in the event the primary power source fails. History of power failures, noting frequency, duration, and, if emergency power

was not available, steps taken to ensure the comfort and well-being of the animals present and the temperature extremes reached in animal rooms during the failure.

Emergency power is available to the vivarium from the Facility Management Utility Department, which has its own power plant and back-up system. Access to the State power grid is also an available option in the event of a failure of the UCLA back-up system. In the event of a planned temperature or environmental condition change (for HVAC system service and-or repair), portable heating/cooling systems are provided by Facility Management and implemented by DLAM when needed. For unplanned events, Vivarium emergency response team and researchers are notified and animal monitoring is increased; portable heating/cooling devices are provided for short term breakdown. If there was an extreme system breakdown for an extended period of time, animals would be relocated to a safer building/zone nearby with functional HVAC system. There has been no power failure in the last 3 years.

2. Other System Malfunctions. If not previously reported, describe animal losses or health problems resulting from power, HVAC, or other life support system (e.g., individually ventilated cages) failures, and mechanisms for reporting such incidences. AAALAC International Rules of Accreditation (Section 2.f).

There have been no animals lost due to power or HVAC failure in the central vivaria in the last 3 years. In January of 2016 and February of 2017, pump failures in 2 aquatics study area rooms for one PI (Sagasti; TLSB, BSRB) resulted in 100+ fish deaths in each

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occurrence. Both instances were reported to the ARC and/or DLAM by lab members.

E. Other Facilities [Guide, pp. 144, 150]

1. Other Animal Use Facilities [Guide, pp. 146-150]Describe other facilities such as imaging, irradiation, and core/shared behavioral laboratories or rooms. Include a description of decontamination and methods for preventing cross-contamination in multi-species facilities.

The ARC Administrator and/or Animal Welfare Coordinator inspect “Research Areas” (i.e., non-housing, non-surgical short-term procedure rooms in which USDA-covered species are not used) at least once every 24 months. Research Areas may be used for procedures such as imaging, irradiation, blood collection, injections, behavioral testing, and/or euthanasia.

All transfers within and between DLAM and these other animal use facilities are subject to review by a DLAM veterinarian and follow our written Biosecurity Policy, which addresses decontamination, movement between facilities, etc.

2. Other Animal Program Support FacilitiesDescribe other facilities providing animal care and use support, such as feedmills, diagnostic laboratories, abattoirs, etc.

Not applicable.

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