1
Running title: HA versus NP readout in influenza virus titration 1
2
3
Detection of non-hemagglutinating influenza A(H3) viruses by 4
ELISA in quantitative influenza virus culture 5
Van Baalen, C.A.1#, C. Els1, L. Sprong1, R. van Beek2, E. van der Vries2, A.D.M.E. Osterhaus1,2 6
and G.F. Rimmelzwaan1,2 7
1 Viroclinics Biosciences, Rotterdam, The Netherlands; 2 Erasmus MC Department of 8
Viroscience, Rotterdam, The Netherlands. 9
10
# Address correspondence to: [email protected] 11
12
Institutional addresses: 13
Viroclinics Biosciences; Marconistraat 16; 3029 AK Rotterdam; The Netherlands. 14
Erasmus MC Department of Viroscience; Dr Molewaterplein 50; 3015 GE Rotterdam; The 15
Netherlands.16
JCM Accepts, published online ahead of print on 12 March 2014J. Clin. Microbiol. doi:10.1128/JCM.03575-13Copyright © 2014, American Society for Microbiology. All Rights Reserved.
on March 21, 2019 by guest
http://jcm.asm
.org/D
ownloaded from
2
Abstract 17
To assess the efficacy of novel antiviral drugs against influenza in clinical trials it is necessary to 18
quantify infectious virus titers in patients’ respiratory tract samples. Typically, this is achieved 19
by inoculating virus-susceptible cells with serial dilutions of clinical specimens, and detecting 20
the production of progeny virus by hemagglutination since influenza viruses generally have the 21
capacity to bind and agglutinate erythrocytes of various species through their hemagglutinin 22
(HA). This readout method is no longer adequate, since an increasing number of currently 23
circulating A(H3) influenza viruses display reduced capacity to agglutinate erythrocytes. 24
Here, we report the magnitude of this problem by analyzing the frequency of HA deficient 25
A(H3) viruses detected in the Netherlands from 1999-2012. Furthermore, we report development 26
and validation of an alternative method to monitor the production of progeny influenza virus in 27
quantitative virus cultures, which is independent of the capacity to agglutinate erythrocytes. This 28
method is based on detection of viral nucleoprotein (NP) in virus culture plates by ELISA, and it 29
produced similar results compared to the hemagglutination assay using strains with good HA 30
activity, including A/Brisbane/059/07 (H1N1), A/Victoria/210/09 (H3N2) and other seasonal 31
A(H1N1), A(H1N1)pdm09 and the majority of A(H3) virus strains isolated in 2009. In contrast, 32
many A(H3) viruses that circulate since 2010 failed to display HA activity and infectious virus 33
titers could only be determined by detecting NP. The virus culture ELISA described here will 34
enable efficacy testing of new antiviral compounds in clinical trials during seasons in which non-35
hemagglutinating influenza A viruses circulate.36
on March 21, 2019 by guest
http://jcm.asm
.org/D
ownloaded from
3
Introduction 37
Efficacy testing of novel antiviral drugs generally involves measuring infectious virus titers in 38
clinical samples at treatment baseline and during follow-up. For influenza, assessment of virus 39
titers by end-point dilution assays commonly relies on the measurement of viral 40
hemagglutination activity in culture supernatants to detect production of progeny virus. 41
However, the continuous accumulation of amino acid substitutions in the viral glycoprotein 42
hemagglutinin (HA) has complicated the detection and characterization of antigenic properties of 43
influenza A(H3N2) viruses by hemagglutination and hemagglutination inhibition (HI) assays, 44
respectively. Poor replicative capacity in Madin-Darby canine kidney (MDCK) cells has been 45
associated with low binding affinities of the viral HA molecules to their receptors (1,13). 46
Reduced receptor binding is also evidenced by failure to agglutinate erythrocytes of various 47
species efficiently, if at all (5,11,13,14,16). Amino acid substitutions in or around the receptor 48
binding site of the HA molecule of A(H3N2) influenza viruses affected the capacity to 49
agglutinate red blood cells (RBC) (13,14,16) and the receptor binding preference has evolved 50
from short, branched sialylated glycans to sialic acids on long polylactosamine chains (5). 51
The replicative capacity of some virus isolates improved upon serial passaging in MDCK 52
cells (1) or MDCK cells that over-express α2,6 SA-Gal receptor (MDCK-siat) (17). This may aid 53
performing HI assays with these viruses to assess their antigenic properties, provided that these 54
remain unaffected during passaging. However, despite additional passages, the frequency of 55
A(H3) virus isolates with impaired HA activity has increased in the Netherlands since 2010, as 56
reported herein. Moreover, serial passaging is no option in clinical trials that require data on 57
infectious virus titers in original clinical specimens. The number of PCR-confirmed samples 58
containing influenza A(H3N2) virus that tested false-negative in quantitative culture assays with 59
on March 21, 2019 by guest
http://jcm.asm
.org/D
ownloaded from
4
HA activity as readout, has also increased since 2010, whereas such discordant results were not 60
found for samples containing influenza A(H1N1) or B viruses (unpublished observations). 61
Thus, alternative methods are required to monitor replication of currently circulating A(H3) 62
viruses in quantitative virus cultures. The viral cytopathic effect (CPE) could be scored, but this 63
procedure lacks specificity, is labor intensive, subjective and not suitable for high throughput 64
applications. Alternatively, viral antigen could be detected in cell culture by ELISA, which is 65
compatible with standardized automated procedures. Although an ELISA has been developed for 66
the measurement of residual virus replication in virus neutralization assays (21,25), it has never 67
been applied for the assessment of virus titers in clinical samples. Here we report the 68
development and validation of an ELISA for the detection of the viral nucleoprotein (NP) in 69
standard 6-day quantitative influenza A virus cultures. We investigated the kinetics of virus 70
replication using the NP-ELISA method, and compared virus titers with those obtained with the 71
conventional HA assay, using laboratory strains and low passage virus isolates with or without 72
good hemagglutination activity. Finally, the performance of both assays for the assessment of 73
infectious virus titers in clinical samples was compared, which indicated that for recent A(H3) 74
influenza viruses the NP-ELISA readout is superior. 75
76
Material and methods 77
Virus strains, virus isolates and clinical specimens. 78
Laboratory strains A/Brisbane/059/07 (H1N1), A/Victoria/210/09 (H3N2) were obtained 79
from the NIBSC (South Mimms, Potters Bar, UK). Epidemic viruses were isolated and 80
propagated in MDCK cells at the National Influenza Center, Erasmus MC, Rotterdam, The 81
Netherlands, as described previously (19), and included the following (sub)types: A(H1N1), 82
on March 21, 2019 by guest
http://jcm.asm
.org/D
ownloaded from
5
A(H1N1)pdm09, A(H3N2) and B, as determined by PCR. One set of respiratory clinical 83
specimens, nasal wash and sputum, was submitted for routine testing for the presence of 84
respiratory viruses at diagnostic unit of the department of Viroscience of the Erasmus MC, 85
Rotterdam, the Netherlands. Approval by the local medical ethical board was obtained before 86
experiments commenced. Informed consent was waived because patient inclusion was performed 87
retrospectively and data were anonymously stored as agreed by the Erasmus MC institutional 88
review board (MEC-2012-599). A second set of clinical specimens, nasopharyngeal swabs, was 89
submitted for the purpose of assessing virus titers as part of clinical trial WP22849 90
(www.clinicaltrials.gov), and appropriate informed consent and ethics approval was obtained. 91
Cells. Madin-Darby Canine Kidney (MDCK) cells were cultured in Eagle minimal 92
essential medium (EMEM) (Lonza, Verviers, Belgium) containing 20 mM Hepes buffer (Lonza), 93
0.075% Na-Bicarbonate solution (Lonza), 2mM L-Glutamine (Lonza), 100 IU/mL Penicillin / 94
100 µg/mL Streptomycin (Lonza), referred to as complete medium (CM), supplemented with 95
10% FBS (Bodinco BV, Alkmaar, The Netherlands). Cells were passaged to new culture flasks 96
twice weekly. One or two days before inoculation cells were seeded in flat-bottom 96-well tissue 97
culture treated microplates (Greiner Bio-one, Alphen a/d Rijn, The Netherlands). 98
HA titer determination. Duplicate serial 2-fold dilutions of 50µL MDCK culture 99
supernatant in PBS were prepared before adding 50µL of 0.5% turkey erythrocyte solution. 100
Following 1 hr incubation at 4°C, the hemagglutination patterns were scored. The reciprocal of 101
the highest dilution showing full agglutination was taken as the HA titer. 102
PCR. Nucleic acids were extracted from 190µL MDCK culture supernatant and eluted to a 103
volume of 110µL by using a MagNApure LC (Roche Diagnostics, Almere, The Netherlands) or 104
QiaSymphony (Qiagen, Venlo, The Netherlands). Before nucleic acid isolation, 10µL phocine 105
on March 21, 2019 by guest
http://jcm.asm
.org/D
ownloaded from
6
distemper virus (PDV) was added as internal control. Cycle time (Ct) values and H1 and H3 106
subtypes were determined by real time RT-PCR on a 7500 Real-Time PCR system (Applied 107
Biosystems, Foster City, CA, USA) or a LightCycler 480 system (Roche Diagnostics, Almere, 108
The Netherlands) as described previously (23). 109
Virus titration. Confluent monolayers of MDCK cells were inoculated with replicate 110
(n=4) serial 10-fold dilutions of virus stocks or clinical samples in 96-well microtiter format in 111
infection medium (IM), which was prepared by supplementing CM with 0.3% Bovine Serum 112
Albumin fraction V (Sigma Aldrich), 2.5µg/mL Amphotericin B (Bristol-Myers Squibb, 113
Woerden, The Netherlands) and Trypsin (Lonza; optimal concentration determined for each lot). 114
After 90 minutes at 37°C in a humidified 5% CO2 incubator, inocula were removed, cells were 115
washed with IM and cultured for 6 days in a humidified 37°C 5% CO2 incubator. Medium 116
control wells (n=12) were included on each plate, and at least two laboratory virus strains with 117
predefined titers were included in each experiment for trending. Results were accepted when 118
titers of trend control viruses were within predefined limits. 119
HA readout. Replication of influenza viruses in cell culture was monitored by measuring 120
hemagglutination activity in the culture supernatants as follows: 25µL undiluted supernatant was 121
mixed with 50µL PBS and 25µL of a 1% turkey erythrocyte solution. After an incubation for one 122
hour at 4°C, hemagglutination patterns were scored, and frequencies of positive and negative 123
wells among the four replicates per dilution were used to calculate virus titers (Log TCID50/mL) 124
according to Spearman-Karber method (6). 125
NP readout. Replication of influenza viruses was also assessed by measuring the 126
production of NP by ELISA as follows: At various time points post inoculation of MDCK cells 127
the cell culture plates were washed once with PBS (Oxoid BR0014G, Fisher Scientific, 128
on March 21, 2019 by guest
http://jcm.asm
.org/D
ownloaded from
7
Landsmeer, The Netherlands), fixed by adding 200µL acetone (80% in water) to each well, and 129
stored at -20°C. After removal of acetone, wells were washed trice with PBS/0.05% Tween20 130
(Merck Millipore, Amsterdam, The Netherlands) before adding the broadly reactive (4,15) 131
influenza A virus NP-specific mouse monoclonal antibody HB65 (EVL Woerden, The 132
Netherlands). Approximately 100 ng of antibody HB65 was added per well in a volume of 200 133
µl PBS containing 2% Skimmed Milk Powder (Sigma 70166) (PBS/SMP). After incubation for 134
one hour at room temperature, the plates were washed three times with PBS/0.05% Tween20 and 135
3 ng of a horseradish peroxidase-labelled Goat-anti-Mouse IgG antibody preparation (Invitrogen, 136
626520) was added in 100uL PBS/SMP and incubated for one hour at room temperature. 137
Following three wash steps with PBS/0.05% Tween20, ready-to-use 3,3’,5,5’-138
tetramethylbenzidine (TMB, Sigma T0440; 100µL/well) was added and plates were incubated at 139
room temperature for 30 minutes before adding 100uL stop solution (1N H2SO4; Sigma 320501). 140
The OD(450-620nm) was measured by using a TECAN F200 plate-reader and signals ≥0.5 were 141
considered positive, and indicative for widespread virus replication. For lower levels of virus 142
replication, e.g. in wells around the endpoint dilution, signals <0.5 but ≥ 0.2 were considered 143
positive when the OD value exceeded three-fold the mean + 3SD of uninfected cell control wells. 144
Because signals above 0.5 also exceeded this latter threshold, scoring of positive and negative 145
wells for TCID50 calculation was effectively based on the latter. Frequencies of positive and 146
negative wells among the four replicates per dilution were used to calculate virus titers 147
(LogTCID50/mL) according to the Spearman-Karber method (6). 148
149
150
151
on March 21, 2019 by guest
http://jcm.asm
.org/D
ownloaded from
8
Results 152
Frequency of virus isolates with poor HA activity in the Netherlands. The annual 153
frequency of influenza A(H3) virus isolates received at the NIC of the Netherlands between 1999 154
and 2012 that agglutinate turkey erythrocytes poorly (HA titers ≤ 2) is shown in table 1. 155
Frequencies increased from ~0%-5% between 1999 and 2003 to ~12-26% between 2004 and 156
2008. The following two seasons were dominated by A(H1N1)pdm09 viruses and only few 157
A(H3N2) isolates were obtained, which all showed low HA activity. During the 2011/2012 158
season, the majority of isolates were of the A(H3) subtype, as determined by RT-PCR, and 159
50.9% (n=162) had HA titers of <2. Isolates with higher HA titers showed no such temporal 160
increase (data not shown). 161
To assess whether low HA activity in the 2011/2012 isolates was due to low virus levels or to 162
poor capacity to agglutinate RBC, we performed PCR, targeting the matrix gene segment, on the 163
samples without HA activity (n=141; one isolate was lost to follow-up) and on those with a HA 164
titer of 2 (n=20). As controls we processed ten isolates obtained during the same season with a 165
HA titer of 4 and ten isolates with a HA titer of 32, in the same experiment. PCR signals 166
indicated the presence of virus (Ct < 40) in two thirds (n=94; 67%) of the 141 isolates without 167
HA activity and in eleven (55%) of the 20 isolates with a HA titer of 2. The remaining cultures, 168
with Ct>40, are likely to have been inoculated with specimens containing non-infectious virus, 169
and were excluded from further analyses with respect to HA activity. 170
PCR-positive isolates with high Ct values are likely to contain insufficient virus for a positive 171
HA result. These samples may represent viruses that have poor intrinsic in vitro replication 172
capacity or that may not be viable for other reasons. The positive control isolates with HA titers 173
of 4 or 32 had median Ct values of 15.5 (range 12.8 – 25.5) and 14.4 (12.8 – 19.2), respectively. 174
on March 21, 2019 by guest
http://jcm.asm
.org/D
ownloaded from
9
As expected, Ct values were generally higher in isolates with HA titers of 2 (16.0 (14.2 – 30.6) 175
or 0 (31.1 (16.0 – 39.0) (Fig. S1). However, 9 (82%) of the 11 PCR positive HA=2 isolates, and 176
21 (22%) of the 94 PCR-positive HA=0 isolates had Ct values that fell within the range of the 177
positive controls. These data indicate that a substantial number of A(H3) virus isolates replicated 178
well in vitro and were HA negative or displayed low HA titers because they failed to agglutinate 179
erythrocytes efficiently. 180
Detection of influenza A virus by NP-ELISA in tissue culture. In order to compare virus 181
replicative capacity with hemagglutination activity more directly, we developed an ELISA for 182
the detection of viral NP in 96-well tissue culture plates. Figure 1 shows NP signals (OD values) 183
of MDCK cultures that had been inoculated with limiting infectious doses of virus A/Vic/361/11 184
per well: With 1:108 and 1:109 diluted virus stock six and one out of eight wells were NP positive 185
respectively, six days post inoculation (dpi 6). The mean OD450-620nm of positive wells increased 186
from ~1.0 at dpi 1 to >2.5 at dpi 6. With a 10-fold higher dose for inoculation (1:107 dilution) all 187
eight wells became positive with mean signals approaching the maximum OD450-620nm level of 188
3.0 already at dpi 1. These signals did not decline up to dpi 6, indicating that the viral NP 189
remained attached to the wells for days, even after viral CPE resulted in complete elimination of 190
the cells. Signals in wells with uninfected control cells were 0.251 ± 0.002 and 0.270 ± 0.003 at 191
dpi 1 and 2, respectively, which declined to 0.007 ± 0.004 at dpi 6. These results are 192
representative for all influenza A viruses that were tested, although kinetics and levels varied 193
among different strains (data not shown). Due to the stability of the NP signal and the favorable 194
signal to noise ratio, detection of NP could provide a reliable alternative to detection of HA 195
activity in culture supernatants for scoring virus-positive and virus-negative cultures in standard 196
virus titration assays. 197
on March 21, 2019 by guest
http://jcm.asm
.org/D
ownloaded from
10
Comparing HA and NP readout for assessing infectious virus titers. To validate the NP-198
ELISA as an alternative readout in virus titrations, we performed three independent experiments 199
with a panel of virus isolates (n=20) with low MDCK passage histories, and the laboratory virus 200
strains A/Bris/059/07 (H1N1) and A/Vic/210/09 (H3N2) as controls (Table 2). Virus titers based 201
on detection of HA activity in the day-6 culture supernatant or NP in the cognate culture plates 202
were similar (i.e. within 1 order of magnitude) for the two laboratory strains, as well as for the 203
five 2008/2009 influenza A(H3) isolates with > 104 TCID50/mL and HA titer of 128 after one in 204
vitro passage. One of the 2008/2009 isolates (#5) had a lower infectious virus titer based on both 205
HA and NP readout: ~0.75 and 2.33 Log TCID50/mL, respectively. The virus titers obtained 206
with the HA and NP-ELISA readouts were similar for all four A(H1N1) isolates tested, including 207
A(H1N1)pdm09, and ranged between 105.17 and 107.08 TCID50/mL. 208
In contrast, A(H3N2) viruses isolated (n=7) between Jul/2009 and Jan/2011 had lower HA 209
titers, and virus titers based on the HA readout were generally lower than those determined with 210
the NP-ELISA. Strikingly, two virus isolates (#7 and #8) with mean virus titers of 10 6.3 211
TCID50/mL based on NP-ELISA readout, scored repeatedly negative when HA activity was 212
used as readout. We confirmed by PCR, that virus was actually present in the supernatants of the 213
NP-positive cultures (data not shown). Collectively, these results indicate that the poor capacity 214
of these virus isolates to agglutinate RBC precluded reliable virus detection and assessment of 215
infectious virus titers. As expected, titers of the three influenza B virus isolates (#18-#20) could 216
be determined by HA assay, but not by NP-ELISA because the detecting antibody used is 217
specific for influenza A virus NP. 218
Performance of the NP-ELISA as readout for the assessment of infectious virus titers in 219
clinical samples. Next, we used the NP-ELISA as readout for determining virus titers in original 220
on March 21, 2019 by guest
http://jcm.asm
.org/D
ownloaded from
11
clinical specimens obtained in the 2011/12 influenza season and compared the results with those 221
obtained with HA activity of the culture supernatants. The samples were submitted for routine 222
diagnostic testing for the presence of respiratory viruses (n=14; Table S1) or collected during a 223
clinical trial designed to evaluate antiviral treatment regimens (n=11; Table S2) between January 224
and May 2012. We tested influenza A(H3) virus PCR-positive samples only, since A(H1) virus 225
titers could be readily determined using the HA assay, which gave identical results as the NP-226
ELISA as readout for all A(H1) titrations performed so far (Table 2 and data not shown). 227
Thirteen out of the 14 original clinical specimens and eight out the 11 clinical trial samples 228
tested positive in the infectious virus titration with NP readout with mean ± SD titers of 3.23 ± 229
0.93 and 3.38 ± 1.08 Log TCID50/mL, respectively. In contrast, no virus was detected by the HA 230
assay in the supernatants of the majority of NP-positive wells, which therefore produced false-231
negative results for twenty of the samples (<0.75 Log TCID50/mL) or lower titers (1.00 Log 232
TCID50/mL; n=1). One out of 14 clinical samples and three out of 11 trial samples tested also 233
negative in the NP-ELISA, indicating that infectious virus titers were below the limit of 234
detection of the virus titration assay. This correlated with the relatively high corresponding Ct 235
values of these specimens. 236
237
Discussion 238
Virological surveillance of influenza in the Netherlands showed that frequencies of A(H3) 239
virus isolates displaying low HA activity increased between 1999 and 2012. Since their 240
introduction in the human population in 1968, A(H3) influenza viruses have evolved 241
continuously. Amino acid substitutions in the HA molecules affected their antigenic properties, 242
in vitro replication and capacity to agglutinate RBC (2,5,7,9,11-14,16,22). A subset of the 243
on March 21, 2019 by guest
http://jcm.asm
.org/D
ownloaded from
12
2011/2012 A(H3) isolates that lacked HA activity, most likely replicated poorly in vitro, as 244
evidenced by high PCR Ct values. However, low virus titers could not explain the absence of HA 245
activity of many other A(H3) virus isolates. Up to 2008, turkey RBC were successfully used as 246
readout in virus titration assays using hemagglutination as readout. During influenza seasons 247
2009/2010 and 2010/2011 A(H1N1)pdm09 viruses were dominant. A(H3) viruses were isolated 248
sporadically, and these isolates agglutinated turkey RBC poorly. Influenza A(H3) viruses with 249
poor HA activity continued to circulate and became the dominant subtype again in the 2011/2012 250
season. The use of RBC from other species, including guinea pig and human, did not consistently 251
improve HA activity for monitoring antigenic drift by HI assays (data not shown). 252
The inefficient hemagglutination activity of influenza virus strains also forms a major 253
problem for the HA readout of quantitative virus cultures of primary specimens in 254
clinical/research settings, as well as in clinical trials. Hemagglutination has long been the 255
preferred readout method because it is generally a simple, fast and reliable virus detection 256
method. It is instrumental as high throughput readout to provide crucial information on the 257
duration of infectious virus shedding and the ability to reduce transmission in efficacy studies of 258
novel antiviral compounds. However the deficiency of virus in primary clinical specimens to 259
agglutinate erythrocytes after the first passage in MDCK cells, precluded the assessment of 260
infectious influenza virus titers by HA readout in the majority of cases during the 2011/2012 and 261
2012/2013 influenza seasons, when A(H3) virus strains were dominant. 262
In order to equip the diagnostic laboratories with a robust HA-independent technique for the 263
detection of progeny virus production in primary quantitative virus cultures, we employed an 264
ELISA that measures NP in multi-well virus culture plates. This NP-ELISA is based on the 265
method described for the WHO-recommended microneutralization assay (21,25). One important 266
on March 21, 2019 by guest
http://jcm.asm
.org/D
ownloaded from
13
difference with virus titration assays is that in neutralization assays cell cultures are inoculated 267
with 100 TCID50/well of known virus strains – after pre-incubation with serial serum dilutions, 268
and virus production is monitored one day after inoculation. To propagate and quantify viruses 269
present in original clinical specimens, other plate types are used and an incubation period of six 270
days is recommended to allow for detection of slowly replicating viruses in wells around the 271
end-point dilution. Therefore, we evaluated the stability of the NP signal up to six days after 272
inoculation, and showed that it increased or remained stable, but never declined. In wells around 273
the end-point dilution, signals generally reached levels that were comparable to those achieved 274
with a 10- to 100-fold higher multiplicity of infection. 275
With HA-competent viruses, the HA and the NP readout methods detected virus replication in 276
largely the same wells and resulted in similar titers. By contrast, infectious virus titers of virus 277
isolates and clinical samples containing HA-deficient viruses could only be determined by using 278
the NP-ELISA. The HA assay may still be preferred as first readout method, since it requires less 279
time and reagents, and it detects A(H1N1), A(H1N1)pdm09 as well as influenza B viruses in the 280
culture supernatants. The tissue culture plates used for determining infectious virus titers can be 281
stored at -20°C until the subtype of the influenza A viruses is identified by PCR, allowing for 282
detection of virus replication by NP-ELISA as second readout in the same titration experiment. 283
Detection of NP relies on the binding of the NP-specific monoclonal antibody HB65 that reacts 284
with a broad range of influenza A viruses (4,15,26), including the A(H1N1) viruses from 1934 285
(A/PR/8/34) and A(H3N2) and A(H1N1)pdm09 viruses isolated in 2012, as reported here. Other 286
recent viruses that were recognized include A/Vic/361/11 (H3N2) and A/Cal/07/09 (H1N1), but 287
also avian and swine influenza viruses A(H5N1), A(H7N7)(15), and H7N9(10). The potential 288
emergence of variants that are not recognized by monoclonal antibody HB65 should be carefully 289
on March 21, 2019 by guest
http://jcm.asm
.org/D
ownloaded from
14
monitored, but based on the documented conservedness of the epitope that is recognized, this is 290
not expected to occur any time soon. Alternatively, a cocktail of monoclonal antibodies could be 291
used to minimize this risk even further. 292
We have tested a number of influenza B virus NP-specific antibody preparations to evaluate 293
ELISA-based detection of influenza B virus-infected cultures at day 6 after inoculation. 294
Although several preparations recognized all Victoria- and Yamagata-lineage strains tested, in 295
many cases signals were too low to distinguish positive and negative wells in a robust way (data 296
not shown). Because current influenza B viruses do agglutinate erythrocytes efficiently, there is 297
no urgent need for alternative readout methods. 298
Antigenic characterization of virus isolates by HI assays form the basis for the annual 299
selection of vaccine strains (2,7). Due to the reduced capacity of A(H3N2) viruses to agglutinate 300
chicken RBCs and, more recently, turkey RBCs, HI data are currently also generated by using 301
mammalian RBC from guinea pig or human. However agglutination patterns are generally more 302
difficult to read, and turkey RBCs are still frequently used for antigenic characterization, 303
possibly leading to underrepresentation of circulating A(H3N2) virus variants for antigenic 304
characterization. Because of the factors that complicate the HI assay, including the need to 305
consider RBC from different species for different virus subtypes, VN assays are now also used 306
for antigenic characterization (18,20,24), and for evaluation of vaccines with relatively low 307
immunogenicity in naive human populations, e.g. H5 and H7 (3,8,21). The ELISA method used 308
in such VN assays detect virus irrespective of their capacity to agglutinate RBCs, a feature that 309
was successfully adapted to improve the monitoring of infectious virus titers in specimens of 310
clinical trials for antivirals. 311
on March 21, 2019 by guest
http://jcm.asm
.org/D
ownloaded from
15
In conclusion, we provided epidemiological data on the emergence of A(H3) influenza viruses 312
that fail to agglutinate erythrocytes efficiently. The HA-deficiency of these viruses complicates 313
monitoring of virus replication in quantitative virus culture and assessment of infectious virus 314
titers in clinical specimens. In order to provide for an HA-independent readout for quantitative 315
virus cultures of primary patient samples in clinical/research and clinical trial settings, we have 316
validated the use of NP detection by ELISA on day six post inoculation of MDCK cells. For 317
currently circulating A(H3) viruses, the HA readout yielded mainly false-negative results, while 318
the NP readout proved to be a robust method that facilitates the measurement of virus titers in 319
clinical specimens, which is critical for the evaluation of new antiviral compounds and therapies 320
in clinical trials. 321
322
Acknowledgments 323
We thank Roche for sharing data on virus titrations of clinical trial specimens. The authors 324
CvB, CE and LS are employed by Erasmus MC spin-out company Viroclinics Biosciences B.V. 325
of which ADMO and GR are consultants. 326
327
Reference List 328
329
1. Asaoka, N., Y. Tanaka, T. Sakai, Y. Fujii, R. Ohuchi, and M. Ohuchi. 2006. Low 330
growth ability of recent influenza clinical isolates in MDCK cells is due to their low 331
receptor binding affinities. Microbes.Infect. 8:511-519. 332
2. Barr, I. G., J. McCauley, N. Cox, R. Daniels, O. G. Engelhardt, K. Fukuda, G. 333
Grohmann, A. Hay, A. Kelso, A. Klimov, T. Odagiri, D. Smith, C. Russell, M. 334
on March 21, 2019 by guest
http://jcm.asm
.org/D
ownloaded from
16
Tashiro, R. Webby, J. Wood, Z. Ye, and W. Zhang. 2010. Epidemiological, antigenic 335
and genetic characteristics of seasonal influenza A(H1N1), A(H3N2) and B influenza 336
viruses: basis for the WHO recommendation on the composition of influenza vaccines for 337
use in the 2009-2010 Northern Hemisphere season. Vaccine 28:1156-1167. 338
3. Cox, R. J., A. S. Madhun, S. Hauge, H. Sjursen, D. Major, M. Kuhne, K. Hoschler, M. 339
Saville, F. R. Vogel, W. Barclay, I. Donatelli, M. Zambon, J. Wood, and L. R. 340
Haaheim. 2009. A phase I clinical trial of a PER.C6 cell grown influenza H7 virus 341
vaccine. Vaccine 27:1889-1897. 342
4. de Boer, G. F., W. Back, and A. D. Osterhaus. 1990. An ELISA for detection of 343
antibodies against influenza A nucleoprotein in humans and various animal species. 344
Arch.Virol. 115:47-61. 345
5. Gulati, S., D. F. Smith, R. D. Cummings, R. B. Couch, S. B. Griesemer, G. K. St, R. G. 346
Webster, and G. M. Air. 2013. Human H3N2 Influenza Viruses Isolated from 1968 To 347
2012 Show Varying Preference for Receptor Substructures with No Apparent 348
Consequences for Disease or Spread. PloS One 8:e66325. 349
6. Karber, G. 1931. Beitrag zur kollektiven Behandlung pharmakologischer Reihenversuche. 350
Exp Pathol Pharmakol 162:480-483. 351
7. Katz, J. M., K. Hancock, and X. Xu. 2011. Serologic assays for influenza surveillance, 352
diagnosis and vaccine evaluation. Expert Rev.Anti.Infect.Ther. 9:669-683. 353
8. Keitel, W. A. and R. L. Atmar. 2009. Vaccines for pandemic influenza: summary of 354
recent clinical trials. Curr.Top.Microbiol.Immunol. 333:431-451. 355
9. Koel, B. F., D. F. Burke, T. M. Bestebroer, d. van, V, G. C. Zondag, G. Vervaet, E. 356
Skepner, N. S. Lewis, M. I. Spronken, C. A. Russell, M. Y. Eropkin, A. C. Hurt, I. G. 357
on March 21, 2019 by guest
http://jcm.asm
.org/D
ownloaded from
17
Barr, J. C. de Jong, G. F. Rimmelzwaan, A. D. Osterhaus, R. A. Fouchier, and D. J. 358
Smith. 2013. Substitutions near the receptor binding site determine major antigenic change 359
during influenza virus evolution. Science 342:976-979. 360
10. Kreijtz, J. H., E. J. Kroeze, K. J. Stittelaar, W. L. de, A. G. van, T. S. van, R. P. van, 361
T. Bestebroer, T. Kuiken, R. A. Fouchier, G. F. Rimmelzwaan, and A. D. Osterhaus. 362
2013. Low pathogenic avian influenza A(H7N9) virus causes high mortality in ferrets upon 363
intratracheal challenge: A model to study intervention strategies. Vaccine 31:4995-4999. 364
11. Kumari, K., S. Gulati, D. F. Smith, U. Gulati, R. D. Cummings, and G. M. Air. 2007. 365
Receptor binding specificity of recent human H3N2 influenza viruses. Virol.J. 4:42. 366
12. Li, Y., D. L. Bostick, C. B. Sullivan, J. L. Myers, S. B. Griesemer, K. Stgeorge, J. B. 367
Plotkin, and S. E. Hensley. 2013. Single hemagglutinin mutations that alter both 368
antigenicity and receptor binding avidity influence influenza virus antigenic clustering. 369
J.Virol. 87:9904-9910. 370
13. Lin, Y. P., X. Xiong, S. A. Wharton, S. R. Martin, P. J. Coombs, S. G. Vachieri, E. 371
Christodoulou, P. A. Walker, J. Liu, J. J. Skehel, S. J. Gamblin, A. J. Hay, R. S. 372
Daniels, and J. W. McCauley. 2012. Evolution of the receptor binding properties of the 373
influenza A(H3N2) hemagglutinin. Proc.Natl.Acad.Sci.U.S.A. 109:21474-21479. 374
14. Medeiros, R., N. Escriou, N. Naffakh, J. C. Manuguerra, and S. van der Werf. 2001. 375
Hemagglutinin residues of recent human A(H3N2) influenza viruses that contribute to the 376
inability to agglutinate chicken erythrocytes. Virology 289:74-85. 377
15. Nicholls, J. M., L. P. Wong, R. W. Chan, L. L. Poon, L. K. So, H. L. Yen, K. Fung, P. 378
S. van, and J. S. Peiris. 2012. Detection of highly pathogenic influenza and pandemic 379
on March 21, 2019 by guest
http://jcm.asm
.org/D
ownloaded from
18
influenza virus in formalin fixed tissues by immunohistochemical methods. 380
J.Virol.Methods 179:409-413. 381
16. Nobusawa, E., H. Ishihara, T. Morishita, K. Sato, and K. Nakajima. 2000. Change in 382
receptor-binding specificity of recent human influenza A viruses (H3N2): a single amino 383
acid change in hemagglutinin altered its recognition of sialyloligosaccharides. Virology 384
278:587-596. 385
17. Oh, D. Y., I. G. Barr, J. A. Mosse, and K. L. Laurie. 2008. MDCK-SIAT1 cells show 386
improved isolation rates for recent human influenza viruses compared to conventional 387
MDCK cells. J.Clin.Microbiol. 46:2189-2194. 388
18. Okuno, Y., K. Tanaka, K. Baba, A. Maeda, N. Kunita, and S. Ueda. 1990. Rapid focus 389
reduction neutralization test of influenza A and B viruses in microtiter system. 390
J.Clin.Microbiol. 28:1308-1313. 391
19. Rimmelzwaan, G. F., M. Baars, E. C. J. Claas, and A. D. M. E. Osterhaus. 1998. 392
Comparison of RNA hybridization, hemagglutination assay, titration of infectious virus and 393
immunofluorescence as methods for monitoring influenza virus replication in vitro. 74:57-394
66. 395
20. Rota, P. A., M. L. Hemphill, T. Whistler, H. L. Regnery, and A. P. Kendal. 1992. 396
Antigenic and genetic characterization of the haemagglutinins of recent cocirculating 397
strains of influenza B virus. J.Gen.Virol. 73:2737-2742. 398
21. Rowe, T., R. A. Abernathy, J. Hu-Primmer, W. W. Thompson, X. Lu, W. Lim, K. 399
Fukuda, N. J. Cox, and J. M. Katz. 1999. Detection of antibody to avian influenza A 400
(H5N1) virus in human serum by using a combination of serologic assays. 401
J.Clin.Microbiol. 37:937-943. 402
on March 21, 2019 by guest
http://jcm.asm
.org/D
ownloaded from
19
22. Smith, D. J., A. S. Lapedes, J. C. de Jong, T. M. Bestebroer, G. F. Rimmelzwaan, A. 403
D. Osterhaus, and R. A. Fouchier. 2004. Mapping the antigenic and genetic evolution of 404
influenza virus. Science 305:371-376. 405
23. Van der Vries, E., J. Anber, A. van der Linden, Y. Wu, J. Maaskant, R. Stadhouders, 406
B. R. van, G. Rimmelzwaan, A. Osterhaus, C. Boucher, and M. Schutten. 2013. 407
Molecular assays for quantitative and qualitative detection of influenza virus and 408
oseltamivir resistance mutations. J.Mol.Diagn. 15:347-354. 409
24. Veguilla, V., K. Hancock, J. Schiffer, P. Gargiullo, X. Lu, D. Aranio, A. Branch, L. 410
Dong, C. Holiday, F. Liu, E. Steward-Clark, H. Sun, B. Tsang, D. Wang, M. Whaley, 411
Y. Bai, L. Cronin, P. Browning, H. Dababneh, H. Noland, L. Thomas, L. Foster, C. P. 412
Quinn, S. D. Soroka, and J. M. Katz. 2011. Sensitivity and specificity of serologic assays 413
for detection of human infection with 2009 pandemic H1N1 virus in U.S. populations. 414
J.Clin.Microbiol. 49:2210-2215. 415
25. WHO. 2011. Manual for the laboratory diagnosis and virological surveillance of influenza. 416
WHO press, Geneva. 417
26. Yewdell, J. W., E. Frank, and W. Gerhard. 1981. Expression of influenza A virus 418
internal antigens on the surface of infected P815 cells. J.Immunol. 126:1814-1819. 419
420
421
422
on March 21, 2019 by guest
http://jcm.asm
.org/D
ownloaded from
20
Figure legends 423
424
FIG 1. NP signals increase up to day 6 post inoculation. MDCK cells were inoculated with serial 425
dilutions of A/Vic/361/11 in 96-well plates (eight replicates per dilution). On days 1, 2 and 6, NP 426
signals were determined by ELISA. Bars are OD450-620nm (mean ± SEM) of positive wells (here 427
defined as > 2-fold above the mean of mock-inoculated cell control (CC) wells) for the -7, -8 and 428
-9 Log diluted virus stock. Numbers of positive wells are above each bar. The CC bars show the 429
OD450-620nm (mean ± SEM) of the eight cell control wells. 430
on March 21, 2019 by guest
http://jcm.asm
.org/D
ownloaded from
21
TABLE 1. Annual frequency of influenza A(H3) clinical isolates with low HA titers
A(H3) isolates (n)
HA = 0 HA = 2 HA ≤ 2
Season n % N % n %
99/00 334 1 0.3 16 4.8 17 5.1
00/01 7 - 0.0 - 0.0 - 0.0
01/02 265 - 0.0 - 0.0 - 0.0
02/03 150 1 0.7 - 0.0 1 0.7
03/04 400 - 0.0 99 24.8 99 24.8
04/05 338 1 0.3 40 11.8 41 12.1
05/06 116 - 0.0 16 13.8 16 13.8
06/07 259 1 0.4 52 20.1 53 20.5
07/08 21 1 4.8 2 9.5 3 14.3
08/09 415 51 12.3 56 13.5 107 25.8
09/10 3 1 33.3 2 66.7 3 100.0
10/11 13 6 46.2 - 0.0 6 46.2
11/12 318 142 44.7 20 6.3 162 50.9
Total 2,639 205 7.8 303 11.5 508 19.2
431
on March 21, 2019 by guest
http://jcm.asm
.org/D
ownloaded from
22
TABLE 2. Virus titers of clinical isolates and laboratory virus strains determined by HA and NP readout
Sample information Log TCID50/ml Means
MDCK passage HA assay NP-ELISA < 1 Log
ID Subtype Datea number HAb Exp.1 Exp.2 Exp.3c mean SD Exp.1 Exp.2 Exp.3 mean SD difference
1 A(H3) Feb/09 1 128 3.75 4.25 nt 4.00 0.35 3.75 4.25 nt 4.00 0.35 y 2 A(H3) Jan/09 1 128 3.25 3.50 nt 3.38 0.18 3.75 4.25 nt 4.00 0.35 y 3 A(H3) Jan/09 1 128 5.00 5.00 nt 5.00 0.00 5.50 6.00 nt 5.75 0.35 y 4 A(H3) Jan/09 1 128 5.50 5.50 5.50 5.50 0.00 6.00 5.75 6.00 5.92 0.14 y 5 A(H3) Jan/09 1 128 <0.75 <0.75 0.75 0.75 - 3.00 1.25 2.75 2.33 0.95 n 6 A(H3) Jan/09 1 128 6.50 6.50 7.00 6.67 0.29 6.50 6.50 7.25 6.75 0.43 y 7 A(H3) Jul/09 1 2 <0.75 <0.75 <0.75 <0.75 - 6.25 6.00 6.75 6.33 0.38 n 8 A(H3) Apr/10 1 0 <0.75 <0.75 <0.75 <0.75 - 6.50 5.75 6.75 6.33 0.52 n 9 A(H3) Dec/10 2 32 3.50 2.25 2.00 2.58 0.80 3.50 4.00 4.00 3.83 0.29 n
10 A(H3) Jan/11 4 4 1.75 1.50 <0.75 1.63 0.18 2.50 3.00 2.75 2.75 0.25 n 11 A(H3) Jan/11 2 8 5.25 4.50 4.75 4.83 0.38 5.75 5.50 4.75 5.33 0.52 y 12 A(H3) Jan/11 4 8 0.75 <0.75 0.75 0.75 0.00 1.50 <0.75 1.25 1.38 0.18 y 13 A(H3) Jan/11 2 8 4.00 3.50 3.75 3.75 0.25 4.25 3.50 4.25 4.00 0.43 y
14 A(H1N1) Jan/09 2 32 5.25 5.00 5.50 5.25 0.25 5.00 5.00 5.50 5.17 0.29 y 15 A(H1N1) Aug/09 2 32 5.25 5.25 5.25 5.25 0.00 5.25 5.25 5.25 5.25 0.00 y 16 A(H1N1)pdm09 Jan/11 2 >32 6.75 7.25 7.25 7.08 0.29 6.75 7.25 7.25 7.08 0.29 y 17 A(H1N1)pdm09 Jan/11 2 >32 7.50 6.75 6.75 7.00 0.43 7.50 6.75 6.75 7.00 0.43 y
18 B Feb/09 1 128 3.75 3.50 3.50 3.58 0.14 <0.75 <0.75 <0.75 <0.75 - n 19 B Mar/11 1 64 6.00 5.75 5.75 5.83 0.14 <0.75 <0.75 <0.75 <0.75 - n 20 B Jan/11 1 >32 5.75 5.50 5.50 5.58 0.14 <0.75 <0.75 <0.75 <0.75 - n
A/Bris/059/07 A(H1N1) NA NA NA 5.75 5.75 5.75 5.75 0.00 5.75 5.75 5.75 5.75 0.00 y A/Vic/210/09 A(H3N2) NA NA NA 5.75 5.25 4.75 5.25 0.50 5.75 5.25 4.75 5.25 0.50 y a Not applicable b HA titers and number of MDCK passages of the virus stocks used in the virus titration experiments. c not tested
432
on March 21, 2019 by guest
http://jcm.asm
.org/D
ownloaded from