Date post: | 11-Dec-2023 |
Category: |
Documents |
Upload: | unisalento |
View: | 0 times |
Download: | 0 times |
Complex Neural Architecture in the Diploblastic Larvaof Clava multicornis (Hydrozoa, Cnidaria)
Stefano Piraino,1* Giuliana Zega,2 Cristiano Di Benedetto,3 Antonella Leone,1,4 Alessandro Dell’Anna,1,2
Roberta Pennati,2 Daniela Candia Carnevali,3 Volker Schmid,5 and Heinrich Reichert5
1Dipartimento di Scienze e Tecnologie Biologiche ed Ambientali, Universita del Salento, 73100 Lecce, Italy2Dipartimento di Biologia, Functional and Reproductive Biology, Universita di Milano, 20133 Milano, Italy3Dipartimento di Biologia, Zoologia e Citologia, Universita di Milano, 20133 Milano, Italy4CNR-ISPA, Campus Ecotekne, 73100 Lecce, Italy5Biozentrum, Neurobiology, University of Basel, 4056 Basel, Switzerland
ABSTRACTThe organization of the cnidarian nervous system has
been widely documented in polyps and medusae, but
little is known about the nervous system of planula
larvae, which give rise to adult forms after settling and
metamorphosis. We describe histological and cytologi-
cal features of the nervous system in planulae of the
hydrozoan Clava multicornis. These planulae do not
swim freely in the water column but rather crawl on the
substrate by means of directional, coordinated ciliary
movement coupled to lateral muscular bending move-
ments associated with positive phototaxis. Histological
analysis shows pronounced anteroposterior regionaliza-
tion of the planula’s nervous system, with different
neural cell types highly concentrated at the anterior
pole. Transmission electron microscopy of planulae
shows the nervous system to be unusually complex,
with a large, orderly array of sensory cells at the ante-
rior pole. In the anterior half of the planula, the basiec-
todermal plexus of neurites forms an extensive
orthogonal network, whereas more posteriorly neurites
extend longitudinally along the body axis. Additional
levels of nervous system complexity are uncovered
by neuropeptide-specific immunocytochemistry, which
reveals distinct neural subsets having specific molecular
phenotypes. Together these observations imply that the
nervous system of the planula of Clava multicornis man-
ifests a remarkable level of histological, cytological, and
functional organization, the features of which may be
reminiscent of those present in early bilaterian animals.
J. Comp. Neurol. 519:1931–1951, 2011.
VC 2011 Wiley-Liss, Inc.
INDEXING TERMS: Cnidaria; Hydrozoa; neuroanatomy; planula; CNS; cephalization; early central nervous system
evolution
A shared feature of Cnidaria and Bilateria is the devel-
opment of a nervous system composed of interconnected
neural cells. In all animal groups, the number of neural
cells, the complexity of their connectivity, and their orga-
nization into regionalized neural assemblies show a great
deal of variation. The evolutionary origin of neuroanatomi-
cal complexity and diversity in eumetazoan nervous
systems represents one of the fundamental problems of
neurobiology. A number of recent comparative develop-
mental and genetic analyses suggest that the nervous
systems of protostomes and deuterostomes arose from a
common evolutionary origin (Lichtneckert and Reichert,
2005, 2008; Denes et al., 2007; Arendt et al., 2008) and
that the urbilaterian nervous system was already a
complex, centralized structure (De Robertis, 2008). Alter-
native views propose multiple, independent evolutionary
origin of central nervous systems (Holland, 2003; Lowe
et al., 2003) and of neuronal types (Moroz, 2009). Since
cnidarians are the evolutionary sister clade of bilaterians
(Collins, 1998; Medina et al., 2001; Ryan et al., 2006;
Dunn et al., 2008), a key question concerns the nature of
a prototype nervous system from which both cnidarian
and bilaterian nervous systems might have evolved. This
Additional Supporting Information may be found in the online version ofthis article.
Grant sponsor: Italian Ministry for Research and Education; Grantnumber: 2007-5WCPWM (to S.P.); Grant sponsor: Swiss National ScienceFoundation (to H.R.).
*CORRESPONDENCE TO: Stefano Piraino, Dipartimento di ScienzeTecnologie Biologiche Ambientali, Universita del Salento, 73100 Lecce,Italy. E-mail: [email protected]
VC 2011 Wiley-Liss, Inc.
Received April 24, 2010; Revised September 18, 2010; AcceptedDecember 30, 2010
DOI 10.1002/cne.22614
Published online February 24, 2011 in Wiley Online Library(wileyonlinelibrary.com)
The Journal of Comparative Neurology | Research in Systems Neuroscience 519:1931–1951 (2011) 1931
RESEARCH ARTICLE
issue is especially interesting in view of recent molecular
developmental data supporting the notion that ancestral
cnidarians already possessed the molecular toolkit nec-
essary to establish a triploblastic and bilateral Bauplan
(Boero et al., 1998, 2007; Finnerty, 2003; Spring et al.,
2002; Seipel and Schmid, 2005; Matus et al., 2006). To
address this question, and thus elucidate the evolutionary
origin of nervous system centralization, new studies on
cnidarian nervous systems that integrate comparative
developmental and neuroanatomical approaches are
needed.
In cnidarians, a great deal of information on structural
organization of the nervous system has been obtained for
adult stages. The nervous systems of both polyps and
medusae are located in both ectodermal and endodermal
cell layers and contain motoneurons, ganglionic inter-
neurons, and sensory cells (the latter mostly within the
ectoderm; for recent reviews see Watanabe et al., 2009;
Galliot et al., 2009). Polyps generally display a ‘‘diffuse’’
epithelial nerve net without morphologically discrete sen-
sory or motor processing centers, except for a localized
ring-like concentration of neural elements around the
mouth (often called the ‘‘head’’ in reports on Hydra). In
swimming jellyfish, a more sophisticated, radially organ-
ized nervous system occurs as single or double nerve
ring at the margin of the umbrella, interconnecting multi-
ple neural cell types and incorporating complex sense
organs (statocysts, ocelli, rhopalia) to form the advanced
neural circuitry required for coordinated movement,
vision, and complex behavioral control (Garm et al.,
2007a,b; Parkefelt and Ekstrom, 2009). The functions of
these neural structures resemble those of the central
nervous system of bilateral animals (Mackie, 2004; Garm
et al., 2006).
In contrast to the detailed knowledge of the nervous
systems in adult cnidarians, little is known about neural
organization in early developmental stages. Cnidarian
ontogeny usually involves a swimming planula larva that,
in response to specific stimuli, settles on the substrate
and metamorphoses into the polyp stage. In Medusozoa,
the polyp stage may give rise to the medusa stage. Many
cnidarian taxa may lack either the polyp or the medusa,
but only in few cases showing direct embryonic develop-
ment into the polyp has the planula stage been sup-
pressed. The presence of neurons in the larva has been
demonstrated in three major cnidarian taxa, namely, the
Anthozoa (Chia and Koss, 1979; Miller and Ball, 2000;
Hayward et al., 2001; Marlow et al., 2009), Hydrozoa
(Martin and Thomas, 1980, 1981; Thomas et al., 1987;
Plickert et al., 1988; Martin, 1992, 2000), and Scyphozoa
(Korn, 1966; Nakanishi et al., 2008; Yuan et al., 2008). In
planulae, the nervous system is located in the ectoderm
and comprises epithelial sensory cells and basally located
ganglionic cells, whose neurites project in a net overlying
the mesoglea (Martin, 1988a,b). In hydrozoans, endoder-
mal stem cells (interstitial cells or i-cells) give rise to
nematoblasts and neuroblasts, which differentiate into
nematocytes and ganglionic cells, respectively, during
their migration toward their final location in the ectoderm.
During the gradual (direct) development of the anthozoan
Nematostella vectensis embryo, a second, endodermal
network of ganglionic cells also appears in late develop-
mental stages (Marlow et al., 2009), linked to the early
onset of polyp-specific structures (pharynx, mesenteries,
and gastric cell populations).
The swimming planulae of some anthozoans and scy-
phozoans possess a specialized ectodermal population of
elongated ciliated cells at the anterior pole, with basal
nuclei, forming the apical organ or apical tuft, a sensory
structure probably involved in perception of chemical
cues at the site of metamorphosis (Widersten, 1968; Chia
and Bickell, 1978; Chia and Koss, 1979; Nakanishi et al.,
2008; Yuan et al., 2008; Marlow et al., 2009). In hydro-
zoan planulae, this structure does not occur.
Most cnidarians have relatively simple, radially sym-
metrical planulae that drift (‘‘swim’’) in the water column
by rotating along the main body axis before settlement
and metamorphosis occur. Within several taxa, however,
non-swimming planulae that display positive geotaxis and
crawl on the bottom have been reported (Otto, 1976;
Hartnoll, 1977; Gerrodette, 1981; Sommer, 1992;
Hellberg, 1995; Orlov, 1996; Heltzel and Babcock, 2002;
Bouillon et al., 2006). Both the ‘‘swimming’’ and the
‘‘crawling’’ movements of planulae are based on ciliary
locomotion (Werner, 1984; Bouillon et al., 2006). The be-
havioral repertoire required for oriented locomotion on
the substrate, however, differs significantly from the rota-
tory activity of ‘‘swimming’’ planulae. The differences in
coordinated behavioral activity of the two types of planula
may be reflected in corresponding differences in the
organization of the nervous system. Indeed, given the
common behavioral constraints encountered by any
animal with benthic (bottom-related) locomotory activity,
it is conceivable that the neurobiological organization of
‘‘crawling’’ cnidarian planulae might be comparable to
that of simple bilaterians with similar behavior.
To investigate both morphological and functional
aspects of this, we focused on the nervous system of the
planula of Clava multicornis (Hydrozoa), a larva with pro-
nounced benthic locomotory activity. Here we report
behavioral observations as well as morphological and neu-
rochemical features of its nervous system. First, behavioral
studies document that the planula shows directed locomo-
tion, with the anterior/aboral pole oriented forward,
accompanied by alternating sideways bending movements.
Second, neuroanatomical observations indicate marked
Piraino et al.
1932 The Journal of Comparative Neurology |Research in Systems Neuroscience
anteroposterior regionalization of the nervous system char-
acterized by a large array of sensory cells at the anterior
pole. Third, immunocytochemical analyses reveal an un-
usual complexity of neural-specific components revealing
distinct cell populations with different molecular proper-
ties. Overall, these findings imply that the presumptive
‘‘simple’’ nervous system of these planulae displays a
surprisingly high level of histological, cytological, and bio-
chemical complexity. Further investigations are needed to
clarify whether the similarities in neural architecture
between cnidarians, including the planulae reported here,
and early bilaterian animals are conserved characters that
were shared by their last common ancestor or whether
they arose from parallel, independent evolution of nervous
systems.
MATERIALS AND METHODS
AnimalsFertile colonies of Clava multicornis (Forskal 1775)
were collected at low tide along Roscoff (France) rocky
shores and transferred to the laboratory. Animals were
reared in aquaria with an open-sea circulation system
(14�C). Daily, some female colonies were isolated,
exposed to light to stimulate planula release, and
checked every hour to collect larvae. Prehatching stages
were obtained by dissection of female gonophores.
The phototropic behavior of planulae was documented
by an image-recording system consisting of a dissecting
microscope (Leica MZ12) equipped with digital photo-
videocamera (Olympus C5050). Newly hatched planula
larvae (12 hours) were kept overnight in the dark before
observation. To observe their behavior, planulae were
transferred into 30-mm glass Petri dishes kept in a water
bath maintained at 14�C. Directed light from a halogen
50-W lamp was provided on one side of the Petri dish
through a fiberglass cable. Images of planula larvae were
taken every 5 seconds to show modifications of body
shape and arranged in series to create a single image.
Light and electron microscopyPlanulae were first anesthetized by short incubation
with 7% MgCl2 and then fixed with 2% glutaraldehyde in
0.1 M cacodylate buffer, pH 7.2. Samples were then post-
fixed with 1% osmium tetroxide in 0.1 M cacodylate
buffer, dehydrated in a graded ethanol series, and em-
bedded in an Epon-Araldite mixture according to standard
transmission electron microscopy (TEM) methods (Maun-
nsbach and Afzelius, 1999). Semithin (1-lm) and ultrathin
(50-nm) sections were cut with a Reichert-Jung Ultracut E
using diamond knives (Diatome Histo and Ultra 45�).
Semithin sections, collected on standard slides and
stained with crystal violet and basic fuchsin, were con-
trolled under a Jenaval light microscope. Ultrathin sec-
tions, collected on 300-mesh copper grids, were stained
with aqueous uranyl acetate and lead citrate (Reynolds,
1963), carbon coated under an Emitech K400X carbon
coater, and observed with a Jeol 100 SX electron micro-
scope. Micrographs were taken directly under the micro-
scope with Kodak 4489 photographic films for TEM.
ImmunohistochemistryPlanulae were fixed in 4% paraformaldehyde (PFA) in
0.1 M phosphate-buffered saline (PBS), pH 7.2, for 1 hour
at room temperature. After rinsing with 0.1 M PBS, fol-
lowed by triplicate washes in 0.4 M glycine, the samples
were stored in 70% ethanol at –20�C. After rehydration,
specimens were incubated with 0.1% Tween-20, 0.25%
Triton X-100 in PBS (PBT) for 30 minutes and then
washed three times for 10 minutes each with PBS. Subse-
quently, samples were blocked with 10% horse serum in
PBT (PBT-HS) for 30 minutes and finally incubated over-
night at 4�C with the different primary antibodies (see
Table 1) diluted in PBT-HS.
After several washes in PBS, samples were incubated
in PBT-HS for 1 hour and then overnight at 4�C with
appropriate secondary (goat anti-rabbit or goat anti-
mouse) antibodies (Alexa Fluor 488 or Alexa Fluor 594
TABLE 1.
Primary Antibodies Used in This Study
Antigen Immunogen Manufacturer, species, type, catalog No. Dilution
Tyrosinatedtubulin
Synthetic peptide (C-terminal amino acids of a-tubulinfrom porcine brain plus an additional N terminallysine and a C-terminal tyrosine; KVEGEGEEEGEEY)
Sigma (Italy), clone TUB-1A2, murine monoclonal,T9028
1:500
Acetylatedtubulin
Purified protein from Strongylocentrotus purpuratus Sigma (Italy), clone 6-11B-1, murine monoclonal,T6793
1:500
GLWamide Synthetic C-terminal-GLWamidated peptide(CAAPPGLW�NH2) coupled via succinimidylm-maleimido-benzoate (MBS) to heyhole limpethemocyanin (KHL)
Gift from Prof. Thomas Leitz (Germany), clone1676IIIp, rabbit polyclonal
1:700
RFamide RF-NH2 coupled via carbodiimide to bovinethyroglobulin
Gift from Prof. Thomas Leitz (Germany), clone1773IIIp, rabbit polyclonal
1:700
Neural complexity in hydrozoan larvae
The Journal of Comparative Neurology | Research in Systems Neuroscience 1933
IgG; Invitrogen, Carlsbad, CA), diluted 1:200–400 in PBT-
HS. Next, the specimens were washed four times in PBS
and mounted in 1,4-diazabicyclo[2,2,2]octane (Dabco,
Sigma Italy) on microscope slides. Immunolabeled speci-
mens were observed via laser scanning confocal
microscopy systems (Leica TCS-NT, Zeiss LSM 510, Zeiss
LSM 5 Pascal). Fluorescence was detected with the com-
binations of 488-nm excitation filter and 530/30-nm
bandpass filter or 530–560 nm excitation filter and 590/
50-nm bandpass filter. Multiple optical sections (0.7–1
Figure 1. Life cycle of C. multicornis. A: Hydroid colony growing on Ascophyllum nodosum (brown seaweed). B: Closeup view of male
polyp: whitish gonophores at different stages of development encircle the hydranth column, just below the tentacles. C: Female polyps
with bright bluish gonophores (embryos at different stages of development). D,E: Female gonophores and embryos at different stages of
development. D: One or two eggs are contained within each gonophore, where fertilization and development take place. E: Sixteen- to
thirty-two-cell embryos (DAPI staining). F: Early larva, 24 hours postfertilization. The anteroposterior axis is already established. G: Hatched
planula. Scale bars ¼ 2 mm in A; 400 lm in B,C; 100 lm in D,G; 60 lm in E,F.
Piraino et al.
1934 The Journal of Comparative Neurology |Research in Systems Neuroscience
lm) were taken through the depth of the specimen
(Z axis), in order to reconstruct 3-D images of the whole
planula. Confocal stack images were recorded and post-
processed with dedicated software. The number and step
size of ‘‘optical sections’’ are given for each image in the
figure legends. Series of optical sections obtained by scan-
ning whole-mount specimens were projected into one
image with greater focal depth. In control samples incu-
bated either with the primary or the secondary antibody
alone, no fluorescent signal or staining was observed.
Antibody characterizationPrimary antibodies (Table 1) raised against tyrosinated
a-tubulin and acetylated a-tubulin were used as pan (gen-
eralized)-neuronal markers, because a-tubulin is a major
components of axonal processes (see Kreis, 1987; Siddi-
qui et al., 1989; Jellies et al., 1996). The tyrosinated
a-tubulin antibody was raised against a synthetic peptide
(T13) containing 11 C-terminal amino acids of a-tubulin
from porcine brain plus an additional N terminal lysine
and a C-terminal tyrosine at the C-terminus (Kreis, 1987).
The acetylated a-tubulin antibody was raised from the
purified protein from the outer arm of the S. purpuratus
(sea urchin) axoneme. Both a-tubulin antibodies recog-
nized a single band at 55 kD on Western blots of total
protein extracts from Clava multicornis polyps. The cross-
phylum specificity of the two antibodies was confirmed
by their consistent pattern of staining in a large number
of metazoan taxa, including cnidarians (Thomas and
Edwards, 1991). In particular, the antiacetylated a-tubulin
antibody has been used as marker of an interphyletically
conserved epitope present in cilia (Piperno and Fuller,
1985) but also for labeling nerve cells and fibers specifi-
cally in different cnidarian taxa (see, e.g., Anthozoa:
Rentzsch et al., 2008; Scyphozoa: Kozmik et al., 2008;
Hydrozoa: Chiori et al., 2009). Similarly, the antityrosi-
nated tubulin antibody has been systematically used as a
neuronal marker in Cnidaria (Groger and Schmid, 2000;
Galliot et al., 2009; Watanabe et al., 2009), with strong
reactivity against motoneuron populations (Nakanishi
et al., 2009, 2010).
Two additional primary polyclonal antibodies directed
against two amidated neuropeptides, GLWamide and
RFamide peptides, were also used (Grimmelikhuijzen,
1985; Leitz et al., 1994). GLWamide and RFamide
antisera were raised and kindly provided by J. Schmich
and T. Leitz (Kaiserslautern). GLWamide controls
(Schmich et al., 1998a,b) were performed by using antise-
rum preadsorbed with He-LWamide II coupled to Hi-Trap
NHS-activated beads (Pharmacia, Freiburg, Germany),
which abolished any staining. The RFamide antiserum
was preincubated with 2 mg/ml bovine thyroglobulin, fol-
lowed by centrifugation to remove antibody populations
specific for the carrier protein (Grimmelikhuijzen, 1985).
Specificity of the polyclonal anti-RFamide antibody has
also been demonstrated in several cnidarian species
(Plickert, 1989; Plickert and Schneider, 2004). In
addition, we have observed colocalization of the 1773IIIp
RFamide antibody staining pattern with the in situ hybrid-
ization labeling pattern for the mRNA of the precursor
protein for neuropeptide Pol-RFamide II in Turritopsis
dohrnii and Hydractinia (Podocoryne) carnea, two hydro-
zoans phylogenetically related to Clava multicornis
(Piraino et al., unpublished data).
Photomicrograph productionDigital images were imported as TIFF files from Leica
or Zeiss software (confocal microscopy) and JEOL TEM
software (electron microscopy) into Adobe Photoshop
and adjusted for optimal brightness and contrast and for
conversion of red-green fluorescent figures into magenta-
green ones.
RESULTS
Development and locomotory behavior ofplanula larvae
The hydroid Clava multicornis (C. multicornis) is a pro-
genetic hydroid without a medusa stage. The embryonic
development of larval planulae takes place on the polyp
colony. When hatched, the planula is worm-like, cigar-
shaped, and approximately 600–800 lm long and has a
prominent anterior pole (club-shaped ‘‘head’’) that tapers
to the posterior pole (‘‘tail’’; Fig. 1G). In contrast to most
planulae, these larvae do not swim in the water column.
C. multicornis planulae instead display a smooth, gliding
movement on the benthos (seaweeds, rocky bottom)
while searching for a suitable site for settlement, where
Figure 2. Phototropic and locomotory behavior of a planula. The hatched larva exhibits positive phototaxis while crawling on the substrate
by alternate left–right bending along the main A-P body axis. Scale bar ¼ 150 lm.
Neural complexity in hydrozoan larvae
The Journal of Comparative Neurology | Research in Systems Neuroscience 1935
within a few days they will ultimately stop, attach by the
anterior end, and develop into primary polyps.
To characterize this locomotory behavior in detail, 50
planulae were placed in Petri dishes individually over 0.5-
mm-graph paper and their movements recorded. The pla-
nulae always moved forward, with the larger, club-shaped
pole ahead. In the presence of light, the planulae were
positively phototactic (Fig. 2). The smooth, anteriorly
directed gliding movement of the planulae was based on
ciliary activity, and it was consistently accompanied by
lateral bending movements with alternate arching along
the main body axis resulting from coordinated myoepithe-
lial contractions (Fig. 2, Supp. Info. Movie 1).
As a result of bending movements propagated from
the anterior end, the planulae displayed consistent
exploratory crawling behavior with alternating sweeps to
the left and right. Occasionally, the front end was transi-
ently lifted off the substrate. Planulae would overcome
small obstacles (e.g., chalk granules) by alternating left-
right bending movements of increasingly wider range
(Supp. Info. Movie 2). When crawling on the substrate,
planulae did not exhibit rotation along the anteroposterior
body axis. For diploblastic planula larvae, these
substrate-bound, forward movements coupled with
alternating lateral bending movements represent com-
plex behavior, which is reminiscent of the undulatory
locomotion patterns of simple bilaterians. These behav-
ioral observations suggest that the nervous system in C.
multicornis planula larvae might be more complex than
that in other cnidarian larval forms. To investigate this,
Figure 3. Microscopic anatomy of C. multicornis planula. A–E: Semithin sections (0.9 lm) A: Longitudinal frontal section at the level of
the endodermal cavity showing diploblastic organization of the planula larva with ectoderm (ec) and endoderm (en) separated by thin mes-
oglea (m). Cnidocytes are visible in the ectoderm and are most numerous at the posterior body pole (asterisks). Anterior pole is to the
left (ic, inner cavity). Boxes I and II correspond to TEM sections shown in Figure 4A,B, respectively. B,C and D,E: Pairs of transverse sec-
tions corresponding to the levels indicated by dashed lines. In each pair, transverse sections are separated by 5 lm, whereas the distance
between pairs is about 30 lm. B,C: Anterior sections showing the initial appearance of an inner lumen; at this level, cirumferential ecto-
derm thickness varies slightly. D,E: At the level of maximum larval circumference, the lumen widens, and ectoderm thickness appears
uniform. In contrast, basiectodermal lacunae associated with the neural plexus are not distributed symmetrically over the mesoglea
(arrows, compare also with Fig. 5D). Scale bars ¼ 50 lm in A; 20 lm in B (applies to B–E).
Piraino et al.
1936 The Journal of Comparative Neurology |Research in Systems Neuroscience
we first carried out a histological analysis of C. multicornis
planulae.
Anterior polarization of the planulabody plan
Histological analysis of planulae revealed their typical
two-layered anatomy, consisting of an external pseudos-
tratified ectoderm and an inner vacuolated endoderm
separated by a thin, acellular mesogleal boundary
(Fig. 3A). A distinctive feature of the ectoderm was its
different thickness at the anterior and posterior poles,
ranging from 55 lm at the anterior to 22 lm at the poste-
rior (Fig. 3A). In addition, transverse sections taken
through the anteriormost part of the planula also revealed
differences in the ectodermal thickness along the body
circumference, whose mean values vary from 41.0 6 1.2
lm to 52.5 6 2.5 lm (Fig. 3B,C). This ectoderm asymme-
try is no longer present at the level at which the anterior
pole attains its maximum width (Fig. 3D,E).
The ectoderm contains several types of specialized cel-
lular elements, including mucous cells and other putative
secretory cells, scattered columnar support cells, and pre-
sumptive sensory cells (Figs. 4A,B, 5A), together with
functional cnidocytes distributed mostly at the posterior
larval end (Fig. 3A). Secretory and sensory cell types were
tightly packed in the anterior ectoderm and showed typi-
cal junctional complexes (Figs. 4A, 5A). Large mucous
cells filled with electron-transparent vesicles together with
numerous other secretory cells were arranged in a dense,
pseudostratified pattern (Figs. 4A,B, 5A). These latter cell
types showed clusters of electron-dense vesicles differing
in shape and size and comparable to the type I and type II
granules described for the larva of Pennaria disticha
Figure 4. Sensory cells in the anterior ectoderm of C. multicornis planula. A: Transmission electron microscopy (TEM) longitudinal section
of the ectoderm corresponding to box I in Figure 3A. In the apical portion of the pseudostratified ectoderm, different cell types are pres-
ent: presumptive supportive cells (sp), large mucous cells (mc) filled with typical granules, a presumptive sensory cell with a dendritic-like
protrusion (sc I; arrow), and a ganglionic cell (gc) in the basal portion of the ectoderm with a large nucleus and a cytoplasm rich in small
granules. This latter cell lies above aligned bundles of neuronal processes of the basiepithelial neural plexus (p). Typical apical junctional
complexes (arrowheads) are evident between different cells. Clear evidence for apocrine secretion is visible distally. B: TEM detail showing
the anterior-lateral area of the ectoderm in longitudinal section corresponding to box II in Figure 3A. Scattered secretory and presumptive
sensory elements (sc II, sc III) are present. The latter form small clusters of two or three sensory cells characterized by an elongated,
polarized shape; heterochromatic nuclei; apical processes (microvilli); scattered cilia (arrowhead); and different types of electron-dense
granules ranging from 150 to 700 nm. Typical secretory cells contain granules and empty vacuoles (asterisks), and some show apoptotic
nuclei (arrow). Scale bars ¼ 4 lm in A; 2 lm in B.
Neural complexity in hydrozoan larvae
The Journal of Comparative Neurology | Research in Systems Neuroscience 1937
(as P. tiarella; Martin and Thomas, 1980; Thomas and
Edwards, 1991). In some cases, morphological evidence
of apocrine secretion could also be detected (Fig. 4A).
A plexus-like, basiepithelial aggregation of putative
neuronal processes was evident in longitudinal sections
of the anterior pole (Figs. 4A, 5B,D,E, 6A). This prominent
anterior plexus was located beneath the ectodermal cell
body layer and was separated from the mesoglea by irreg-
ular basal protrusions of the ectodermal cells (Fig. 5D). In
the basal region, close to the plexus, both the support
cells and the mucous cells showed large phagosomes
containing degenerating organelles and apoptotic nuclei
(Fig. 4A,B). The support cells themselves were not easily
distinguishable either because they were hidden and
compressed by other large and more prominent cellular
elements or because they often shared some of the mor-
phological features of gland cells. Myoepithelial cells
whose basally elongated contractile elements lie above
the mesogloea were also found in the larval ectoderm.
Their contractile apparatus showed aligned thin and thick
filaments and scattered Z-elements but did not appear to
be organized in a regular pattern (Fig. 5F).
Presumptive sensory cells were elongated, showing a
heterochromatic nucleus located centrally and a promi-
nent nucleolus. These cells had a rather dense cytoplasm
rich in organelles, including mitochondria, a well-
developed Golgi, numerous parallel RER cisternae, and
abundant glycogen granules. The cytoplasm was charac-
terized by numerous granules, differing in electrondensity
from strong to moderate, and of three size ranges (small,
�150–200 nm; medium, �400 nm; large, �750 nm;
Figs. 4B, 5A). A first type of presumptive sensory cell (sc
I), although rarely observed, was characterized by a club-
shaped, prominent swelling (Fig. 4A), resembling the mor-
phology of the bulb-shaped dendritic portion of the olfac-
tory cells in mammals (see Donini et al., 1998). A second
type of vesicle-rich, presumptive sensory cell (sc II) pos-
sessed a long cilium arising from a pit with an apical open-
ing (Figs. 4B, 5G). In the apical cytoplasm of these cells,
several granules were concentrated sometimes close to
the outer surface and suggesting exocytosis to the pit
lumen. A third type of presumptive sensory cell (sc III)
had apical portions with protrusions or short microvilli,
(Figs. 4B, 5A,C). These sensory cells were spaced regu-
larly, either singly or in characteristic multicellular associ-
ations, in which at least one cell with small granules was
associated with one cell with large granules between the
tightly packed glandular cells (Fig. 5A). The slender basal
processes of these presumptive sensory cells extended
into the anterior basiectodermal plexus (Fig. 4A,B).
Scattered nonciliated ganglion cells were detected in a
basal position above the mesoglea among packed and
aligned bundles of putative neuronal processes (Fig. 4B).
They were filled with microtubules, mitochondria, and elec-
tron-dense neurosecretory granules (about 8–10 nm in
diameter; Fig. 5E). These cells were characterized by a large
nucleus with a prominent nucleolus and finely granular
cytoplasm. The ectoderm was characterized by the pres-
ence of typical junctional complexes (septate junctions
associated with zonulae adherentes) between adjacent
cells (Figs. 4A, 5A,C,G). The occurrence of gap junctions on
lateral cell membranes, located halfway through the thick-
ness of ectoderm, was indicated by microinjections and
incubation assays with fluorescent dyes of different molec-
ular weights (Leone, unpublished data).
The endoderm of planulae consisted of highly vacuo-
lated cells with a loose epithelial organization (Fig. 6B).
Differentiating cnidoblasts (Fig. 6C) were more abundant
near the posterior pole. These endodermal cells were on
the whole comparable in morphology to the other hydro-
zoan larvae (Thomas and Edwards, 1991), with abundant
cytoplasmic inclusions (phagosomes, secretory and yolk
Figure 5. TEM section of planula ectoderm pattern and structure. A: Longitudinal section of pseudostratified anterior ectoderm. Putative
sensory cells (sc) are clustered among large cells (mc) and are characterized by large heterocromatic nuclei localized in their midapical por-
tion and several mitochondria. Sensory cell clusters contain cells with granules of three different sizes. In the apical portion of the ecto-
derm, junctional complexes are clearly visible (arrowheads). B: Semithin longitudinal horizontal section of the anterior pole. A prominent
neural plexus is detected as an arc at the base of the ectoderm (arrows); a narrow gap in the mesoglea is often observed at the anterior
pole of the larva (arrowhead). C: Apical portion of presumptive sensory cells (sc III), with protrusions by short microvilli emerging from the
ectodermal surface. The cytoplasm contains several dark granules and some mitochondria. D: Electron micrograph showing the arrangement
of the nerve plexus (p) with respect to the basal processes of ectodermal cells and the mesoglea (m). A thick bundle of neuronal processes
(seen both in longitudinal and in transversal sections) lies over a series of thin columnar cell protrusions, interspersed by lacunae (l). Mito-
chondria are present in both neurites and lacunae. The basal processes of ectodermal cells are in contact with the mesogleal layer, which
acts as a basal lamina. E: Enlargement of neuronal processes in longitudinal section showing bundles of microtubules (arrowhead). F: Detail
of the basal portion of the ectoderm showing the presence of clear contractile elements (arrow) forming a wide domain of a myoepithelial
cell; thin and thick filaments are visible. G: Detail of the apical portion of a sensory cell (sc II) showing a prominent cilium arising from
within a cleft or pit, surrounded by granule-rich cytoplasm. The basal apparatus consisting of a typical cnidarian rootlet and of proximal and
distal centrioles (arrows) is readily distinguishable. The cells are connected by junctional complexes formed by septate junctions followed
by zonulae adherents (arrowheads). Scale bars ¼ 5 lm in A; 25 lm in B; 1 lm in C; 2 lm in D,F; 500 nm in E,G.
Neural complexity in hydrozoan larvae
The Journal of Comparative Neurology | Research in Systems Neuroscience 1939
granules, empty vacuoles; Fig. 6B,C). In transverse and
longitudinal sections, the endoderm showed a narrow
central lumen throughout the length of the planula (Figs.
4A, 6A–C). Longitudinal sections revealed a gap in the
mesoglea close to the anterior pole corresponding to an
interruption of the ectodermal layer, leaving the endo-
derm cells in contact with the outer environment
(Fig. 6D,E). Near this mesogloeal discontinuity, the endo-
dermal lumen became distinguishable (Fig. 6D,E). Loose
cell contacts within the central epithelium, allowing
exchange of fluid and small particles (<100 lm) between
the inner cavity and the external medium via a funnel-
shaped ectodermal area, were revealed by short-term
(2 hours) incubation experiments of planulae with dyes or
GFP-conjugated particles (Leone et al., unpublished data).
To investigate the organization of the presumptive sen-
sory cells and neural processes of the planula in more
detail, we adopted a complementary immunocytochemical
approach. Both pan-neuronal and nerve cell-specific
markers were used in this study.
Figure 6. Planula ectoderm and endoderm. A: Semithin transverse section at the anterior pole. The main neural plexus (arrowheads) lies
above the basal cytoplasmic processes of ectodermal cells. In transverse sections, it forms an arc, extending for perhaps one-third of the
anterior circumference. The thin mesoglea and vacuolated endoderm (en) encircle the inner cavity (ic). B: Thin transverse section showing
details of the developing inner cavity (ic). Many ciliary processes can be seen still enclosed in cytoplasmatic portions, and the apical cyto-
plasm (ac; arrowheads) may be close to being discharged. Junctional complexes between the cells (arrows) are clearly seen in the subapi-
cal region. C: Thin transverse section. Typical vacuolated and ciliated cells line the planula’s internal cavity, in which several cilia are
visible in cross-section (arrowheads). Ciliogenesis has been completed, and the cavity is much more pronounced. Differentiation of endo-
dermal cnidoblasts (arrow) is complete. Various dense granules and phagosomes (ph) are interspersed within the endoderm cells. D: Semi-
thin longitudinal horizontal section through the anterior pole of a planula. The mesoglea (delimited by dashed lines) presents a gap, and
here endodermal cells reach the outer surface (arrow). E: TEM detail of the area in D showing the gap area in the mesoglea and ectoderm.
A few endodermal cells are directly exposed to the environment here (arrow). Scale bars ¼ 25 lm in A,D; 4 lm in B,C; 10 lm in E.
Piraino et al.
1940 The Journal of Comparative Neurology |Research in Systems Neuroscience
Architecture of the planula nervous systemThe architecture of the entire nervous system of the
planula was studied first by immunocytochemical labeling
of whole mounts with antisera against two pan-neuronal
markers, the tyrosinated a-tubulin (TT) and the acetylated
a-tubulin (AT; Piperno and Fuller 1985; Kreis, 1987; Siddi-
qui et al., 1989; Jellies et al., 1996). In both cases, whole-
mount analyses revealed a striking polarization of the
nervous system in that sensory cells and nerve fibers
were restricted almost exclusively to the anterior half of
the planulae (Fig. 7A,B). Spindle-shaped sensory cells
were located in a spatially restricted, cap-like arrange-
ment at the anterior pole (Fig. 7A), with apical processes
reaching the planula’s outer surface and basal neurites
projecting toward an extensive basiectodermal neural
plexus (Fig. 7B,C). The anteriormost part of this plexus
consisted of densely arranged fiber bundles that pro-
jected in an orthogonal, rectilinear manner, whereas, in
Figure 7. Immunohistochemical analysis of planula nervous system with antityrosinated tubulin (TT) and antiacetylated a-tubulin antibod-
ies (AT). A: Whole mount of a TT-immunostained planula (sum of 12 optical sections) revealing a highly developed neural network at the
anterior pole. The TT-immunoreactive system shows ectodermal sensory elements concentrated in the anterior first one-fourth of the
larva together with orthogonal commissural pathways, which in the second one-fourth of the body crosses obliquely the main A-P axis at
a 45� angle. Additional TT-immunoreactive elements located in the posterior half of the larva were identified via light microscopy as cni-
docysts. B,C: Planulae labeled by AT immunoreactivity. Labeling is seen in the outer cilia (oc), localized all over the planula ectodermal
surface, and in the internal endodermal cilia (ic) within the lumen. B: Sum of five optical horizontal sections at the level of the inner
lumen. Several elongated cells are labeled in the anterior ectoderm, partially clustered in lateral groups (circled; lc, lateral cells). Gangli-
onic cells are also scattered over the median and posterior regions (gc). A basiectodermal nerve plexus lines the mesoglea and appears
thicker at the anterior pole (first one-fourth of planula). Note the anterior discontinuity of mesoglea (arrowhead). C: Sum of five optical
horizontal sections at the base of the ectoderm. Numerous spindle-shaped cells labeled in the anterior ectoderm connect to the nerve
plexus, whose fibers are organized in an orthogonal network. The anteriormost gap in the mesoglea is paralleled by a looser organization
of the nerve plexus. D: AT immunoreactivity in a prehatching planula (36 hours postfertilization; sum of five optical horizontal sections)
shows the early appearance of sensory elements and commissural elements orthogonal to the main body axis. The gonophore peduncle
(at the top of the embryo shows a large number of protective cnidocytes and ciliated cells. Scale bars ¼ 45 lm in A,B; 40 lm in C; 30
lm in D.
Neural complexity in hydrozoan larvae
The Journal of Comparative Neurology | Research in Systems Neuroscience 1941
the rearmost part of the plexus, these bundles formed a
more oblique arrangement (Fig. 7A,C). The dense neural
plexus ended at approximately half the distance along the
anteroposterior axis. In the posterior half of the planula,
only a few longitudinal TT-immunoreactive fibers were
seen. The only other TT-immunoreactive cells in the pos-
terior half were nonneuronal cnidocytes, which were
more concentrated at the posterior pole of the planula
(Fig. 7A), where the mouth of the primary polyp develops
at metamorphosis.
The analysis of optical sections of planulae immunola-
beled with antiacetylated a-tubulin revealed sensory cells
restricted to the larval anterior pole and neural processes
that projected into the neural plexus (Fig. 7B,C). The
arrangement of the sensory cells and the organization of
the associated neural plexus were regular and highly or-
dered, with two notable exceptions. First, narrow, denser
clusters of AT-immunoreactive cells were detected in the
anterior ectoderm, where these cells appeared to be
more concentrated than elsewhere (Fig. 7B, dashed
Figure 8. GLWamide-immunoreactive nervous system of planulae. Localization of GLWamide peptides in whole mounts. A: Color-depth
code localization (sum of 12 optical horizontal sections) of GLWamide-immunoreactive cells. A dense three-dimensional array of ectoder-
mal sensory cells characterizes the anterior pole of the planula. From each peripheral cell body, a thin cytoplasmatic process extends
proximally. B: In the posterior part of the planula, GLWamide-immunoreactive neurons run longitudinally along the border between ecto-
derm and endoderm. These presumptive ganglionic interneurons might also have a sensory function, insofar as their cell bodies may
extend to the surface. C,D: Anterior region of planula enlarged. C: A single optical section close to the top surface of the planula.
D: Same specimen as in C. A single optical section of the planula head (top view) at the median point along the Z-axis shows that GLW-
amide cells are absent from the centralmost area of the ectoderm, i.e., at the mesogleal disruption shown in Figures 5 and 6. E: Enlarge-
ment of a bipolar ganglion cell from the posterior region of the planula. Punctate immunolabeling F: C. multicornis embryo 24 hours post-
fertilization with low or no signals of GLWamide immunoreactivity (same as Fig. 1F). G: C. multicornis embryo 36 hours postfertilization.
After establishment of the A-P body axis, differentiation of GLWamide-immunoreactive cells is seen at the anterior pole of the future
planula. Scale bars ¼ 40 lm in A,F; 35 lm in B; 30 lm in C,D; 5 lm in E; 45 lm in G.
Piraino et al.
1942 The Journal of Comparative Neurology |Research in Systems Neuroscience
circles). These clusters appeared not to be labeled by the
TT antiserum. Second, the neural plexus had a fascicular
organization at its most anterior tip, which was disrupted
at the narrow area where the discontinuity in the meso-
glea was detected by TEM microscopy (Fig. 7B,C). This
feature was revealed only by AT immunolabeling. AT-im-
munoreactive sensory cells and neural fibers were rarely
observed in the posterior half of the planula (Fig. 7B), con-
firming the findings obtained in the whole-mount assays
using the anti-TT antibody.
Because acetylated a-tubulin is a major component of
axonemes, immunolabeled cilia were also observed
arising from the ectoderm cell layer or into the inner
endoderm lumen (Fig. 7B). AT-immunoreactive cells were
detectable in the embryonic nervous system soon after
the establishment of the primary body axis (from 18 to 24
hours postfertilization; Fig. 7D).
Localization and morphology of GLWamide-immunoreactive neurons
The use of specific antibodies for cnidarian neuropepti-
des showed that the global pan-neural pattern obtained
by the TT and AT immunolabeling can be separated mor-
phologically into component subpatterns covering differ-
ent neural types. We screened first for cells that were
immunolabeled by polyclonal antibodies for the GLWa-
mide neuropeptide family, which are characterized by
Figure 9. RFamide-immunoreactive nervous system of planulae. A: Whole-mount localization of RFamide-immunoreactive system (sum of
12 optical horizontal sections) reveals presumptive sensory neurons encircling the anterior end of the planula and bipolar ganglionic cells
with longitudinally oriented neurites showing punctate immunolabeling. B: Enlargement of the anterior end of the planula. RF-immunoreac-
tive sensory cells appear in a narrow belt, mainly as two opposing clusters and with a few located at the anterior pole. Their cell bodies
are situated basally or within the ectoderm and have cytoplasmic processes extending distally and proximally. A commissural plexus of
RFamide-positive neurite bundles is situated between the ectoderm and the extracellular matrix, linking the two lateral clusters of sensory
cells transversely. C: Enlargement of RFamide-immunoreactive sensory cell, with typical club-shaped, short apical process and basal neu-
rite. D: Enlargement of a bipolar ganglionic cell from the posterior pole. E: Differentiating RFamide-immunoreactive cells in C. multicornis
embryo 36 hours postfertilization, when A-P polarity is already established. Posterior ganglionic cells project a single neurite anteriorly.
Scale bars ¼ 40 lm in A; 25 lm in B; 10 lm in C; 3 lm in D; 30 lm in E.
Neural complexity in hydrozoan larvae
The Journal of Comparative Neurology | Research in Systems Neuroscience 1943
the C-terminal aminoacid sequence -Gly-Leu-Trp-NH2
(Leitz et al., 1994). These peptides play an important role
as neurotransmitters in cnidarians, but they have been
also found in mammals, in which they have a presumptive
role in sensory mechanisms (Hamaguchi-Hamada et al.,
2009). Two distinct types of GLWamide-positive cells were
found in C. multicornis planulae (Fig. 8A–E).
The first consists strikingly of up to 80 GLWamide-
immunoreactive cells densely packed at the anterior
pole of the planula (Fig. 8A). In the anteriormost part
of the ectoderm, the pattern of these GLWamide-
immunoreactive cells shows an overlap with TT- and
AT-immunoreactive cells (Fig. 7A–C). A depth-coded pro-
jection series of confocal sections indicates that a signif-
icant number of GLWamide-immunoreactive cells are
regularly arranged in a dome-shaped array at the front
end of the planula (Fig. 8A). The posterior border of this
neuronal cupola of GLWamide-immunoreactive cells
corresponds approximately to the level of the anterior
neural plexus. The elongated, club-shaped cells show
features typical of sensory cells observed by TEM; they
extend apically toward the outer surface and project
a long basal neurite into the anterior neural plexus
(Fig. 8C,D). At the apex of the GLWamide-immunoreac-
tive dome, a small gap in the array of sensory cells corre-
sponds to the mesogleal gap beneath the funnel-shaped
area described above (Fig. 8D).
A second type of GLWamide-immunoreactive neurons
is observed in the middle and posterior parts of the pla-
nula behind the anterior neural plexus (Fig. 8B,E). These
cells are less abundant, and their distribution within the
ectoderm is rather sparse. They become rare toward the
posterior pole of the planula and are hardly detectable in
the tail end (Fig. 8B). In contrast to the anterior GLWa-
mide cell population, these bipolar neurons have short
somata that are basally embedded in the ectoderm and
are associated with two longitudinal neurites, which pro-
ject anteriorly to the neural plexus and posteriorly to the
planula tail (often manifesting punctate immunolabeling;
Fig. 8E). These cells are also detected by the TT and AT
antisera. Based on their number, arrangement, and
ectodermal location, as well as form of perykarya, neurite
morphology, and projection patterns, this second type of
GLWamide-immunoreactive cell most likely corresponds to
the basally located ‘‘ganglionic’’ cells previously described
from other hydrozoan planulae (Martin, 1988a,b).
The GLWamide-immunoreactive neural cells of the pla-
nula are first detected in the embryonic ectoderm 24–36
hours after fertilization, when the anterior-posterior
polarization in the embryo is already clearly established
(Fig. 8F,G). The GLWamide neural system is already fully
organized when the planula detaches from the mother
polyp and begins its locomotory activity.
Localization and morphology ofRFamide-immunoreactive neurons
RFamide immunolabeling also reveals two morpho-
logically distinct types of neural cells in the planula
ectoderm: presumptive sensory neurons and neurons with
longitudinally oriented fiber processes (Fig. 9A). However,
the number and the distribution pattern of these RFamide-
immunoreactive cells are distinctly different from those of
GLWamide-immunoreactive cells. First, RFamide-immuno-
reactive neurons are markedly fewer (20–25) than GLWa-
mide-immunoreactive cells (Fig. 9A,B). Second, most
RFamide-immunoreactive cells are localized in a narrow
belt encircling the ‘‘head’’ of the planula (Fig. 9A,B).
Furthermore, they appear to be clustered mostly into two
main groups on opposing sides; few scattered cells are
oriented toward the forefront of the planula or between
the two main clusters along the narrow belt (Fig. 9B).
These cells apparently are not labeled by the TT antise-
rum; however, they may correspond to the narrow clusters
labeled by the AT antiserum. The most anterior RFamide-
immunoreactive cells show typical features of sensory
neurons. They are club-shaped with a short apical process
extending to the outer surface of the planula and a longer
basal neurite-like process projecting toward the anterior
plexus (Fig. 9C). RFamide-immunoreactive cells of the sec-
ond type (Fig. 9D) have short somata scattered along the
main body axis with two opposing basal neurites running
above the mesoglea toward the anterior and posterior
poles. They show an orderly pattern of parallel distribution
along the anteroposterior axis (Fig. 9A). Like the
GLWamide-immunoreactive cell population, cells of the
RFamide-immunoreactive neural system are apparent in
the embryonic ectoderm (Fig. 9E) by the time when the
main planula body axis is established at 24 hours postfer-
tilization. Both anteriorly clustered sensory neurons and
neurons with longitudinal projecting fibers are detected
in 24–36 hours postfertilization embryos (Fig. 9E). At
the time of release from the mother polyp, the RFamide-
positive neural system is fully differentiated in the planula.
DISCUSSION
In contrast to the planktonic planulae of many cnidar-
ians that perform simple ciliary swimming behavior
(Werner, 1984; Bouillon et al., 2006), the benthic planu-
lae of C. multicornis carry out relatively complex, sub-
strate-bound, directed locomotion. This crawling behavior
is characterized by the forward orientation of the planu-
la’s anterior end, usually accompanied by lateral bending
movements that help the animal to progress on the sub-
strate. Such coordinated locomotory activity requires a
relatively complex nervous system, which must develop
during embryogenesis, insofar as it is completed and
already functional when a planula hatches. The anterior
pole of the larva is especially important for rapid sensing
Piraino et al.
1944 The Journal of Comparative Neurology |Research in Systems Neuroscience
of the structure and suitability of the substrate. The
anterior end is highly polarized anatomically and corre-
spondingly displays dense aggregates of specific types of
neural cells. The ultrastructural analysis revealed in the
C. multicornis planula the occurrence of chemical
synapse-like structures with asymmetric distribution of
synaptic vescicles (not shown), suggesting a polarized
conduction of signal in one direction, as observed in
anthozoan planula larvae (Chia and Koss, 1979). More-
over, functional and molecular evidence demonstrated
the occurrence of gap junction communication channels
with critical roles both in the sensory-motor integration/
homeostasis of C. multicornis larvae and in the control of
signaling pathways driving larval morphogenesis (Leone
et al., unpublished data).
Our analysis of the planula larva of C. multicornis
reveals a remarkably high degree of anterior neuroana-
tomical specialization. This is expressed in 1) the number
and types of sensory neurons concentrated in the ante-
rior ectoderm and 2) the characteristic localization of a
prominent anterior neural plexus. Both of these morpho-
logical features are likely to be prerequisites for the for-
ward-directed locomotory behavior of the planula. The
complementary concentration of mucous gland cells at
the anterior pole provides a useful specialization for tran-
sient adhesion of the larva as it crawls on the substrate
and for its final settlement at metamorphosis (Bouillon,
1995). Given that the gland cells are in basal contact with
the neural plexus or embedded between sensory
elements, the extent of mucous secretion could possibly
be regulated by neural control.
Anterior polarization of the larval nervoussystem
A striking feature of anterior neural polarization in pla-
nulae of C. multicornis is the large number of sensory
cells in a densely arranged, dome-shaped domain. This
orderly arrangement of sensory cells is especially appa-
rent in GLWamide-immunoreactive labeled preparations.
A comparable degree of neural concentration has yet not
been observed in any other cnidarian planulae.
In terms of the anatomical complexity, the nervous sys-
tems of most cnidarian planulae comprise a radially
organized, diffuse network that is distributed throughout
the swimming larva (see Galliot et al., 2009). Integrated
into this network are scattered groups of sensory cells
(mainly at the anterior pole) and nematocytes (mainly at
the posterior or ‘‘oral’’ end, where the polyp mouth will be
formed at metamorphosis). In planulae of Aurelia, an RFa-
mide neural network has been shown to be regionalized
along the A-P axis in a graded plexus with regularly
spaced neurons in the anterior domain and longitudinal
neurites extending toward the aboral pole (for up to 60%
of the body length), whereas TT-immunoreactive cells
appear quite homogeneously distributed (Nakanishi
et al., 2008; Galliot et al., 2009). In planulae of Acropora,
RFamide-immunoreactive cells were found to be more
densely distributed along the anterior larval half but did
not manifest any recognizable clustered organization
(Hayward et al., 2001). In the early planula of Nematos-
tella, RFamide-immunoreactive cells appear to be
scattered in the ectoderm, with a higher concentration
localized near the ciliary apical tuft, and later in develop-
ment corresponding cells are manifest at the base of the
developing tentacles of the primary polyp (Marlow et al.,
2009; Galliot et al., 2009).
According to Thomas and Edwards (1991), ‘‘. . . neither
sensory organs [n]or a concentration of neural elements
has been demonstrated in the hydrozoan planulae.’’ A few
studies of nervous system development in hydrozoan pla-
nulae have been carried out. In the hydrozoan Podocor-
yne carnea, modular units composed of ring-like belts of
ectodermal nerve cells begin to differentiate from the
anterior toward the posterior larval pole starting at
24 hours postfertilization to form a diffuse network
(Groger and Schmid, 2001). The 24-hour planula of the
hydrozoan Pennaria disticha has been shown to possess a
subpopulation of ganglionic FMRFamide-immunoreactive
cells (Martin, 1988a,b), whose cell bodies and neurites
form a basal plexus in the ectoderm confined to the ante-
rior half of the planula. Sensory cells appear initially at
the anterior pole and later in development extend along
the entire length of the planula (Martin, 1988b). Both
LWamide neurosecretory and RFamide-immunoreactive
nerve cells were observed in the anterior parts of both
developing and mature larvae of Hydractinia echinata
(Plickert, 1989; Leitz and Lay, 1995; Gajewski et al.,
1996). The spatial distribution pattern of the GLWamide-
immunoreactive system, however, has been documented
so far only in Hydractinia echinata polyps and larvae
(Schmich et al., 1998a,b). In this species GLWamide-
immunoreactive sensory cells are scattered radially in the
ectoderm; in the anterior part of the planula, they are
localized subapically in a belt 150 lm wide (see Gajewski
et al., 1996: Fig. 3A,B; and Schmich et al., 1998b:
Fig. 2C). This arrangement contrasts with the majority
of GLWamide-immunoreactive cells in the planulae of
C. multicornis, which are markedly polarized in a
restricted domain in the foremost part of the planula
head (Fig. 8A).
Thus while a modest degree of regionalization has
been reported for the nervous system of other planulae,
in none of these is the neural architecture comparable to
the highly clustered organization observed in C. multicor-
nis. Moreover, none of the cnidarian planulae investigated
so far show the circumferential distribution of sensory
Neural complexity in hydrozoan larvae
The Journal of Comparative Neurology | Research in Systems Neuroscience 1945
cells around a frontal gap in the ectoderm (Figs. 6D,E,
8A,C,D). Although an anterior enrichment of sensory and
ganglionic cells is known for most planulae, the types and
number of sensory cells and their degree of clustered
localization in C. multicornis planulae are unparalleled.
The array of anterior sensory cells appears to comprise
diverse types. Based on their ultrastructural features, at
least three putative sensory cell types can be identified
with distinct apical structures and differing cytoplasmic
content (granules of different sizes and electron density).
Some of these are also characterized by the expression
of specific neuropeptides. Indeed, a clear subdivision of
the large, seemingly homogeneous population of anterior
sensory neurons becomes apparent in comparing GLWa-
mide-immunoreactive and RFamide-immunoreactive cells
(Figs. 8, 9). Whereas GLWamide immunoreactivity reveals
a large apical dome of sensory cells, immunoreactivity for
the RFamide peptide is shown only by a restricted belt of
sensory neurons that mostly form two contralateral cell
groups at the front pole of the planula. Given the cylindri-
cal appearance of the planula and the current notion of
radial symmetry in cnidarians, this latter observation is
remarkable. A comparison of the two sets of GLWamide-
labeled and RFamide-labeled cells with the total cell
population labeled by pan-neural cell markers indicates in
addition the existence of further, as yet unidentified neu-
ral cell subpopulations. For example, the neural elements
that are responsible for the extensive rectilinear network
of (TT-immunoreactive) commissural fibers in the anterior
part of the planula remain to be identified.
The arrays of sensory cells are probably chemo- or
photoreceptors involved in key events such as settlement
and metamorphosis. Neuropeptides secreted from sen-
sory cells are thought to represent important internal
signals for the coordination of the metamorphic process
in cnidarians (Schwoerer-Bohning et al., 1990; Leitz,
1993; Schmich et al., 1998a,b; Plickert et al., 2003) as
well as for the synaptic transmission of neuronal activity
(Watanabe et al., 2009). High levels of neuropeptide
immunoreactivity have been found in nervous systems of
planulae in a number of cnidarian species. In the hydro-
zoan Hydractinia echinata, small, anterior neural clusters
immunoreactive for GLWamide and/or RFamide are
thought to be involved in the detection of chemical cues,
in the control of locomotory and phototropic behavior,
and in the initiation of metamorphosis (Plickert, 1989;
Leitz and Lay, 1995; Schmich et al., 1998a,b; Muller and
Leitz, 2002; Katsukura et al., 2004). After discovery of
metamorphosin A, various other GLWamides have
been isolated from adult hydrozoans and anthozoans
(for review see Leitz, 1998), and the occurrence of
GLWamide-immunoreactive cell populations has been
documented in the neural system of several cnidarians,
including anthozoans, scyphozoans, and hydrozoans
(Leitz et al., 1994; Leitz and Lay, 1995). Their putative
function is in chemical reception and as an activation
signal for the metamorphic process. The existence of a
novel mammalian neuropeptide related to the cnidarian
GLWamide family and perhaps involved in sensory mech-
anisms has recently been documented (Hamaguchi-
Hamada et al., 2009). Several reports indicate the ability
of GLWamide peptides to induce metamorphosis in planu-
lae belonging to different taxa, from corals to hydroids
(Leitz and Lay, 1995; Iwao et al., 2002; Muller and Leitz,
2002; Plickert et al., 2003). In view of these findings, it is
conceivable that the GLWamide-immunoreactive cells of
C. multicornis might be directly involved in the initiation
and/or signaling regulation of this process. Both
GLWamide-immunoreactive and RFamide-immunoreactive
neurites exhibited punctate immunolabeling patterns
(Figs. 8A,B,E, 9A), a common feature of cnidarian peptider-
gic systems that is thought to reflect multiple releasing
sites of neuropeptides along the length of the neurites
(see Parkefelt and Ekstrom, 2009, and references therein).
Given the pronounced positive phototactic behavior of
planulae of C. multicornis, at least some of the anterior
sensory cells are likely to be photoreceptors. In particular,
the RFamide-immunoreactive cells might be involved in
light detection. Although the detailed mode of function of
the RFamide peptide family in cnidarians remains to be
clarified (Watanabe et al., 2009), reports on the larvae of
Hydractinia echinata and young medusae of Tripedalia
cystophora suggest a role in transmission of photic
stimuli (Katsukura et al., 2004; Plickert and Schneider,
2005). Martin (2004) has suggested an interaction
between opsins and RFamide peptides in photoreceptors
of Cubozoa. This last observation seems to be confirmed
in Hydrozoa by the colocalization of RFamide peptides in
cells expressing the CropJ opsin in Cladonema radiatum
medusae (Suga et al., 2008).
RFamide-immunoreactive sensory cells and their
neurites have been reported to be diffusely distributed in
the anterior half of ‘‘swimming/rotating’’ anthozoan pla-
nulae (Hayward et al., 2001; Marlow et al., 2009). Mature
‘‘swimming/drifting’’ planulae of the scyphozoan Aurelia
furthermore possess an anteriorly concentrated ectoder-
mal nervous system with an apical, lateral distribution
pattern of RF-immunopositive cells and an apical plexus
extending toward the posterior end (Nakanishi et al.,
2008). Compared with the FMRFamide-immunoreactive
nervous system of the Aurelia planula, however, the num-
ber of apical sensory cells in that of C. multicornis
appears to be greater, and these are located in a nar-
rower belt and are clustered mostly into two contralateral
domains. Phototactic behavior comparable to that of
C. multicornis planulae has been reported in the planula
Piraino et al.
1946 The Journal of Comparative Neurology |Research in Systems Neuroscience
of H. echinata, which, while creeping forward, bends the
front end through the axis of light direction, exposing the
previously shaded side toward the light source and stimu-
lating bending in the opposite side. In this context, the
two lateral clusters of RFamide-immunoreactive cells in
C. multicornis planulae might be involved in photorecep-
tion and/or transmission of the light stimuli to the myoe-
pithelial cells that mediate bending of the body. Further
experiments will shed light on the presumptive sensory
functions of these cells and the molecular basis for photo-
reception in C. multicornis planulae.
Whereas the role of RFamides has been associated
with specific sensory functions such as photoreception
and with specific behaviors such as phototaxis, the neural
signaling related to phototactic behavior and the role of
GLWamide in planulae of C. multicornis and in cnidarians
generally are not yet understood. The marked differences
in spatial pattern and number of GLWamide-immunoreac-
tive vs. RFamide-immunoreactive cells in planulae of
C. multicornis support the notion that the nervous system
of these planulae is remarkably highly developed, com-
prising multiple populations of neuronal cells with differ-
ent morphological and biochemical properties. Whether
coexpression of GLWamide and RFamide occurs in a
restricted subset of these cells has not yet been deter-
mined and remains to be investigated, but the distinctive
patterns of distribution of these two neural cell popula-
tions suggest a discrete localization for each peptide.
An unusually complex neural plexus is found in the
anterior part of this planula (Fig. 10). It comprises a highly
Figure 10. Diagram of the nervous system of C. multicornis planulae. The anterior pole is at the top in both the drawing and the picture.
GLWamide immunoreactive (GLWamide-ir) cells are in magenta, RFamide immunoreactive (RFamide-ir) cells in green. Nonpeptidergic, tyro-
sin-/tubulin-immunoreactive nervous fibers are in blue. Scale bar ¼ 100 lm in photograph.
Neural complexity in hydrozoan larvae
The Journal of Comparative Neurology | Research in Systems Neuroscience 1947
ordered array of circumferential, oblique, and longitudinal
neurite fiber bundles. The neurites of the sensory cells
project into this network of bundles, so many of the
processes in the plexus may convey sensory information.
Neurites that arise from scattered ganglionic cells in the
posterior part of the planula appear also to project into
the anterior plexus. This implies that the anterior plexus
may be involved in the integration of neural information
from different parts of the planula. In planulae of other
hydrozoans, a diffuse ectodermal neural plexus extending
to the entire length of the planula has already been
described (Martin, 1988a,b; Leitz, 1993; Groger and
Schmid, 2001), but, in terms of neurite number, diversity,
polarization, and pattern of arrangement, the level of
structural and organizational complexity of the neural
plexus of the larvae of C. multicornis seems to be
unmatched.
Evolutionary considerationsIn its overall arrangement, the regularly spaced and
highly concentrated array of diverse sensory cells at the
front end of the planula is reminiscent of the sensory
neuronal arrays of simple bilaterians (Raikova et al., 1998;
Gaerber et al., 2007; Kotikova and Raikova, 2008;
Schmidt-Rhaesa, 2009). Moreover, the ordered array of
neural processes in this plexus has morphological features
that are also found in the central neuropiles of bilaterian
ganglia (Meinertzhagen, 2010). For example, the occur-
rence near the anterior (cephalic) pole of multiple longitu-
dinal fiber bundles intersected orthogonally by commis-
sural fiber bundles is a characteristic feature of the central
nervous system of some simple protostomes (Nielsen,
1994). Given its high level of morphological complexity,
the anatomical restriction of the anterior neural plexus to
one side of the planula along a secondary body axis
(orthogonal to the AP main axis) in theory would be suffi-
cient to result in the formation of a structure with most of
the features of a simple bilaterian central nervous system.
It is currently not known whether this type of hypothetical
‘‘dorsoventral’’ restriction of the anterior plexus occurs in
any cnidarian planulae, but the circumferential asymmetry
in thickness observed in the ectoderm of the anteriormost
region of planulae of C. multicornis might be considered to
support the hypothesis of an early establishment of a
primordial dorsoventral patterning mechanism.
A further feature of the anterior neural plexus in the
planulae of C. multicornis planula is reminiscent of the
properties of anterior central ganglia in protostomes. In
the planula, circumferential GLWamide-immunoreactive
neurite bundles of the anterior neural plexus are distrib-
uted around a frontal gap in the ectoderm and mesoglea,
where the endoderm bulges out is in contact with the
external environment. This condition is comparable to the
circumferential organization of RFamide-immunoreactive
and GLWamide-immunoreactive cells and neurites sur-
rounding polyp hypostomes (Grimmelikhuijzen, 1985;
Schmich et al., 1998a; Martin, 2000). In protostomes,
neurite bundles of the anterior neural ganglia form
circumferential connectives encircling the anterior esoph-
agus. Hence, in both cases, elements of the anterior
nervous system are formed and assembled around a
cylindrical nonneural domain. To our knowledge, this is
the first observation of an anatomical orifice in the ante-
rior pole of a hydrozoan planula larva at the opposite end
from the so-called oral pole, where the mouth of the
primary polyp will be formed on metamorphosis. The
functional role of this histological discontinuity requires
further investigation. The observation of a ciliated endo-
dermal epithelium lining the inner cavity prompted the
hypothesis that effective communication with the outer
environment might exist. If so, the cilia might be required
for the circulation of water, comparable to circulatory
mechanisms observed within the endodermal canals of
small hydromedusae (Roosen-Runge, 1967). Preliminary
experiments (Leone, unpublished observations) corrobo-
rate the hypothesis of a functional orifice by demonstrat-
ing exchange of fluids and particles between the inner
planula cavity and the surrounding environment.
Taken together, all of these organizational features
imply that the nervous system of C. multicornis planula is
characterized by a remarkable level of complexity whose
features are reminiscent of those found in simple bilater-
ian animals. What might be the evolutionary origin of this
complexity? Two possibilities can be envisaged. First, the
relative complexity of the nervous system in planulae
might have evolved as an adaptation to a benthic life style
and in response to the needs of substrate-based direc-
tional locomotion. In this case, the nervous system of
C. multicornis planulae would reveal the evolutionary and
developmental potential of a cnidarian-specific radial Bau-
plan to generate nervous system complexity. Second, the
relative complexity of the nervous system of C. multicornis
planulae might indicate that the common ancestor of cni-
darians and bilaterians had already attained a degree of
ancestral neural ‘‘cephalization.’’ In this case, the nervous
system of C. multicornis planulae might reflect organiza-
tional and developmental features that in extant bilater-
ians characterize the assembly of a brain-like centralized
nervous system. The two hypotheses are not mutually
exclusive: the adaptation of nervous systems to a benthic
life style might follow in consequence of the activation of
preexisting genetic mechanisms for anterior nervous sys-
tem polarization and concentration. Given the limited
knowledge about the ecology and neuroanatomy of the
larval stages in most cnidarians, further investigations of
cnidarian larvae displaying a benthic locomotory behavior
Piraino et al.
1948 The Journal of Comparative Neurology |Research in Systems Neuroscience
comparable that of the planulae of C. multicornis should
indicate whether the occurence of an anterior concentra-
tion (‘‘cephalization’’) of the nervous system is a plesio-
morphic or apomorphic larval character.
Although the notion that cnidarians are derived from a
bilateral ancestor is controversial, there is undisputed evi-
dence that cnidarians and bilaterians share an extensive
developmental genetic toolkit leading to axial patterning,
neural specification, and triploblasty in protostome and
deuterostome lineages (Kusserow et al., 2005; Boero
et al., 2007; Jacobs et al., 2007). Whether this common
developmental toolkit is used in a cnidarian-specific way
to build the cnidarian nervous system or it is used accord-
ing to a basic ur-Eumetazoan pattern to generate the
nervous systems of all animals remains an open question.
There has been considerable debate in the literature
about the origin of the cnidarian oral–aboral and directive
body axes and how they relate to bilaterian anteroposte-
rior and dorsoventral axes (Martindale, 2005; De Jong
et al., 2006; Rentzsch et al., 2006; Ball et al., 2007). A
major difficulty lies in the uncertain equivalence of Hox/
Parahox gene expression patterns in different cnidarians
(Yanze et al., 2001; Finnerty et al., 2003). On the other
hand, the finding of a conserved role of the Wnt family sig-
naling in axis formation supports the idea of oral–aboral
determination having common ancestry in cnidarians and
bilaterians (Guder et al., 2006; Momose et al., 2008).
Planulae of the hydrozoan C. multicornis possess
several morphological specializations that differ from
those of the larval stages of traditional cnidarian model
systems. Among these are an anterior opening, directed
bilateral locomotion, and primitive ‘‘cephalization’’ at the
anterior end. Its overall morphology presents key features
that have been suggested as plesiomorphic requisites of
a planuloid ancestor of cnidarians and bilaterians
(Hyman, 1951; Holland, 2003). In this respect and in view
of the occurrence of a mouth-like anterior discontinuity, it
is difficult to define the functional anterior pole of a C.
multicornis planulae as the ‘‘aboral’’ pole. The current
oral–aboral controversy is probably linked to a polyp-
focused anatomical terminology, which should probably
be abandoned. It has already been noted that the ecto-
derm and endoderm of planulae cannot be assumed to
be developmentally equivalent in different species of
cnidarians and also that gene expression patterns in
planulae of different cnidarian taxa must be compared
with caution (Yuan et al., 2008). Moreover, modes of
gastrulation and developmental timing are so diversified
in cnidarian embryos and larvae (Bouillon, 1995) that
class- or phylum-level generalizations should not be
based on single model observations. Similarly, the
clustered anterior nervous system in planulae of C.
multicornis should not be interpreted per se as a
‘‘protobrain’’-equivalent structure. However, one should
not rule out the possibility that, by anticipation of sexual
maturity (progenesis) in a cnidarian-prototype ancestral
larva, further C. multicornis-like anatomical adaptations
for creeping bilateral locomotion (including a centralized
nervous system) might have been retained and become
specialized further, thus breaking down most evolutionary
constraints linked to the anatomies of both polyp and
medusa. Additional comparative studies on new models
of cnidarian/early bilaterian relationships will be required
to address these issues and to test the hypothesis that
the prototypal neuroanatomical condition of a common
ancestor from which extant cnidarian and bilaterian nerv-
ous systems derived had already attained a high level of
organizational complexity.
ACKNOWLEDGMENT
This article is dedicated to the late Volker Schmid
(Basel), who deeply inspired this work. Ferdinando Boero
(Lecce) encouraged and offered valuable advice on earlier
versions of the manuscript. We thank T. Leitz (Heidelberg)
for kindly providing the neuropeptide antibodies, Elisa
Giangrande (Lecce) for laboratory assistance, and Elaine
A. Robson (Reading) for English revision. Fabio Tresca
(Lecce) offered technical support for preparation of
figures. We appreciate the hospitality offered by Patrick
Cormier at the Station Biologique de Roscoff. We also
thank the anonymous reviewers whose detailed com-
ments improved this article.
LITERATURE CITEDArendt D, Denes AS, Jekely G, Tessmar-Raible K. 2008. The
evolution of nervous system centralization. Phil TransR Soc Lond B Biol Sci 363:1523–1528.
Boero F, Gravili C, Pagliara P, Piraino S, Bouillon J, Schmid V.1998. The cnidarian premises of metazoan evolution: fromtriploblasty, to coelom formation, to metamery. Ital J Zool65:5–9.
Boero F, Schierwater B, Piraino S. 2007. Cnidarian milestonesin metazoan evolution. Integr Comp Biol 47:693–700.
Bouillon J. 1995. Classe des Hydrozoaires. In: Grasse PP, Dou-menc D, editors. Traite de zoologie, vol 3. Paris: Masson.p 29–416.
Bouillon J, Gravili C, Pages F, Gili JM, Boero F. 2006. An intro-duction to Hydrozoa. Mem Mus Nat Hist Natur Paris 194:1–591
Chia FS, Bickell L. 1978. Mechanisms of larval settlementand the induction of settlement and metamorphosis: areview. In: Chia FS, Rice ME, editors. Settlement andmetamorphosis of marine invertebrate larvae. New York:Elsevier. p 1–12.
Chia FS, Koss R. 1979. Fine-structural studies of the nervoussystem and the apical organ in the planula larva of thesea-anemone Anthopleura elegantissima. J Morphol 160:275–298.
Collins AG. 1998. Evaluating multiple alternative hypothesesfor the origin of Bilateria: an analysis of 18S rRNAmolecular evidence. Proc Natl Acad Sci U S A 95:15458–15463.
Neural complexity in hydrozoan larvae
The Journal of Comparative Neurology | Research in Systems Neuroscience 1949
De Robertis EM. 2008. Evo-devo: variations on ancestralthemes. Cell 132:185–195.
Denes AS, Jekely G, Steinmetz PR, Raible F, Snyman H, Prud’-homme B, Ferrier DE, Balavoine G, Arendt D. 2007. Molec-ular architecture of annelid nerve cord supports commonorigin of nervous system centralization in Bilateria. Cell129:277–288.
Donini SD, Branduardi P, Campiglio S, Candia Carnevali MD.1998. Localization of calcitonin gene-related peptide mRNAin developing olfactory axons. Cell Tissue Res 294:81–91.
Dunn CW, Hejnol A, Matus DQ, Pang K, Browne WE, SmithSA, Seaver E, Rouse GW, Obst M, Edgecombe GD,Sorensen MV, Haddosk SH, Schmidt-Rhaesa A, Okusu A,Kristensen RM, Wheeler WC, Martindale MQ Giribet G.2008. Broad phylogenomic sampling improves resolutionof the animal tree of life. Nature 452:745–749.
Finnerty JR. 2003. The origins of axial patterning in the Metazoa:how old is bilateral symmetry? Int J Dev Biol 47:523–529.
Finnerty JR, Paulson D, Burton P, Pang K, Martindale MQ.2003. Early evolution of a homeobox gene: the parahoxgene Gsx in the Cnidaria and the Bilateria. Evol Dev 5:331–345.
Gaerber CW, Salvenmoser W, Rieger RM, Gschwentner R.2007. The nervous system of Convolutriloba (Acoela) andits patterning during regeneration after asexual reproduc-tion. Zoomorphology 126:73–87.
Gajewski M, Leitz T, Schlossherr J Plickert G. 1996. LWamidesfrom cnidaria constitute a novel family of neuropeptideswith morphogenetic activity. Roux Arch Dev Biol 205:203–242.
Galliot B, Quiquand M, Ghila L, De Rosa R, Milijkovic-Licina M,Chera S. 2009. Origin of neurogenesis, a cnidarian view.Dev Biol 332:2–24.
Garm A, Ekstrom P, Boudes M, Nilsson DE. 2006. Rhopaliaare integrated part of the central nervous system in boxjellyfish. Cell Tissue Res 325:333–343.
Garm A, O’Connor M, Parkefelt L, Nilsson DE. 2007a. Visuallyguided obstacle avoidance in the box jellyfish Tripedaliacystophora and Chiropsella bronzie. J Exp Biol 210:3616–3623.
Garm A, Poussart Y, Parkefelt L, Ekstrom P, Nilsson DE.2007b. The ring nerve of the box jellyfish Tripedalia cysto-phora. Cell Tissue Res 329:147–157.
Gerrodette T. 1981. Dispersal of the solitary coral Balanophylliaelegans by demersal planula larvae. Ecology 62:611–619.
Grimmelikhuijzen CJP. 1985. Antisera to the sequenceArg-Phe-amide visualize neuronal centralization in hydroidpolyps. Cell Tissue Res 241:171–182.
Groger H, Schmid V. 2001. Larval development in Cnidaria: aconnection to Bilateria? Genesis 29:110–114.
Guder C, Philipp I, Lengfeld T, Watanabe H, Hobmayer B,Holstein T. 2006. The Wnt code: cnidarians signal the way.Oncogene 25:7450–7460.
Hamaguchi-Hamada K, Fujisawa Y, Koizumi O, Muneoka Y,Okado N, Hamada S. 2009. Immunohistochemical evi-dence for the existence of novel mammalian neuropeptidesrelated to the Hydra GLW-amide neuropeptide family. CellTissue Res 337:15–25.
Hartnoll RG. 1977. Reproductive strategy in two British speciesof Alcyonium. In: Ceidigh PO, Boaden PJS, editors. Biology ofbenthic organisms. New York: Pergamon Press. p 321–328.
Hayward DC, Catmull J, Reece-Hoyes JS, Berghammer H,Dodd H, Hann SJ, Miller DJ, Ball EE. 2001. Gene structureand larval expression of cnox-2Am from the coral Acroporamillepora. Dev Genes Evol 211:10–19.
Hellberg ME. 1995. Stepping-stone gene flow in the solitarycoral Balanophyllia elegans: equilibrium and nonequilibriumat different spatial scales. Mar Biol 123:573–581.
Heltzel PS, Babcock RC. 2002. Sexual reproduction, larvaldevelopment and benthic planulae of the solitary coralMonomyces rubrum (Scleractinia: Anthozoa). Mar Biol 140:659–667.
Holland ND. 2003. Early central nervous system evolution: anera of skin brains? Nat Rev Neurosci 4:617–627.
Hyman LH. 1951. The invertebrates, vol 2. Platyhelminthesand Rhynchocoela: the acoelomate bilateria. New York:McGraw-Hill. p 1–572.
Iwao K, Fujisawa T, Hatta M. 2002. A cnidarian neuropeptide ofthe GLWamide family induces metamorphosis of reef-buildingcorals in the genus Acropora. Coral Reefs 21:127–129.
Jacobs DK, Nakanishi N, Yuan D, Camara A, Nichols SA, Har-tenstein V. 2007. Evolution of sensory structures in basalmetazoa. Integr Comp Biol 47:712–723.
Jellies J, Kopp DM, Johansen KM, Johansen J. 1996. Initial for-mation and secondary condensation of nerve pathways inthe medicinal leech. J Comp Neurol 373:1–10.
Katsukura Y, Ando H, David CN, Grimmelikhuijzen CJP,Sugiyama T. 2004. Control of planula migration by LWa-mide and RFamide neuropeptides in Hydractinia echinata.J Exp Biol 207:1803–1810.
Korn H. 1966. Zur ontogenetischen Differenzierung derCoelenteratengewebe (Polyp-Stadium) unter besondererBerucksichtigung des Nervensystems. Z Morphol OkolTiere 57:1–118.
Kotikova EA, Raikova OI. 2008. Architectonics of the centralnervous system of Acoela, Platyhelminthes, and Rotifera.J Evol Biochem Physiol 44:95–108.
Kreis TE. 1987. Microtubules containing detyrosinated tubulinare less dynamic. EMBO J 6:2597–2606.
Kusserow A, Pang K, Sturm C, Hrouda M, Lentfer J, SchmidtHA, Technau U, von Haeseler A, Hobmayer B, MartindaleMQ, Holstein TW. 2005. Unexpected complexity of theWnt gene family in a sea anemone. Nature 433:156–160.
Leitz T. 1993. Biochemical and cytological bases of metamor-phosis in Hydractinia echinata. Mar Biol 116:559–564.
Leitz T. 1998. Metamorphosin A and related compounds: anovel family of neuropeptides with morphogenic activity.Ann N Y Acad Sci 839:105–110.
Leitz T, Lay M. 1995. Metamorphosin-A is a neuropeptide.Roux Arch Dev Biol 204:276–279.
Leitz T, Morand K, Mann M. 1994. Metamorphosin-A: a novelpeptide controlling development of the lower metazoanHydractinia echinata (Coelenterata, Hydrozoa). Dev Biol163:440–446.
Lichtneckert R, Reichert H. 2005. Insights into the urbilaterianbrain: conserved genetic patterning mechanisms in insectand vertebrate brain development. Heredity 94:465–477.
Lichtneckert R, Reichert H. 2008. Anteroposterior regionaliza-tion of the brain: genetic and comparative aspects. AdvExp Med Biol 628:32–41.
Lowe CJ, Wu M, Salic A, Evans L, Lander E, Stange-ThomannN, Gruber CE, Gerhart J. 2003. Anteroposterior patterningin hemichordates and the origins of the chordate nervoussystem. Cell 113:853–865.
Mackie GO. 2004. Central neural circuitry in the jellyfish Aglan-tha: a model ‘‘simple nervous system.’’ Neurosignals 13:5–19.
Marlow HQ, Srivastava M, Matus DQ, Rokhsar D, MartindaleMQ. 2009. Anatomy and development of the nervous sys-tem of Nematostella vectensis, an anthozoan cnidarian.Dev Neurobiol 69:235–254.
Martin VJ. 1983. A fine structural study of metamorphosis ofthe hydrozoan Mitrocomella polydiademata. J Morphol 176:261–287.
Martin V. 1988a. Development of nerve cells in hydrozoanplanulae. I. Differentiation of ganglionic cells. Biol Bull 174:319–329.
Piraino et al.
1950 The Journal of Comparative Neurology |Research in Systems Neuroscience
Martin V. 1988b. Development of nerve cells in hydrozoanplanulae: II. Examination of sensory cell differentiationusing electron microscopy and immunocytochemistry. BiolBull 175:319–329.
Martin VJ. 1992. Characterization of a RFamide-positive sub-set of ganglionic cells in the hydrozoan planular nerve net.Cell Tissue Res 269:431–438.
Martin VJ. 2000. Reorganization of the nervous system duringmetamorphosis of a hydrozoan planula. Invertebr Biol 119:243–253.
Martin VJ, Thomas MB. 1980. Nerve elements in the planulaof the hydrozoan Pennaria tiarella. J Morphol 66:27–36.
Martin V, Thomas MB. 1981. Elimination of the interstitialcells in the planula larva of the marine hydrozoan Pennariatiarella. J Exp Zool 217:303–323.
Matus DQ, Pang K, Marlow H, Dunn CW, Thomsen GH, Martin-dale MQ. 2006. Molecular evidence for deep evolutionaryroots of bilaterality in animal development. Proc Natl AcadSci U S A 103:11195–11200.
Maunnsbach AB, Afzelius BA. 1999. Biomedical electronmicroscopy. London: Academic Press.
Medina M, Collins AG, Silberman JD, Sogin ML. 2001. Evaluat-ing hypotheses of basal animal phylogeny using completesequences of large and small subunit rRNA. Proc NatlAcad Sci U S A 98:9707–9712.
Meinertzhagen I. 2010. The organisation of invertebratebrains: cells, synapses and circuits. Acta Zool 91:64–71.
Miller DJ, Ball EE. 2000. The coral Acropora: what it cancontribute to our knowledge of metazoan evolution andthe evolution of developmental processes. Bioessays 22:291–296.
Momose T, Derelle R, Houliston E. 2008. A maternally local-ised Wnt ligand required for axial patterning in the cnidar-ian Clytia hemisphaerica. Development 135:2105–2113.
Moroz LL. 2009. On the independent origins of complexbrains and neurons. Brain Behav Evol 74:177–190.
Muller WA, Leitz T. 2002. Metamorphosis in the Cnidaria. CanJ Zool 80:1755–1771.
Nakanishi N, Yuan D, Jacobs DK, Hartenstein V. 2008. Earlydevelopment, pattern, and reorganization of the planulanervous system in Aurelia (Cnidaria, Scyphozoa). DevGenes Evol 218:511–524.
Nakanishi N, Hartenstein V, Jacobs DK. 2009. Development ofthe rhopalial nervous system in Aurelia sp. (Cnidaria,Scyphozoa) Dev Genes Evol 219:301–317.
Nakanishi N, Yuan D, Hartenstein V, Jacobs DK. 2010.Evolutionary origin of rhopalia: insights from cellular-levelanalyses of Otx and POU expression patterns in the devel-oping rhopalial nervous system. Evol Dev 12:404–415.
Nielsen C. 1994. Larval and adult characters in animal phylog-eny. Am Zool 34:492–501.
Orlov DV. 1996. The role of larval settling behavior in determi-nation of the specific habitat of the hydrozoan Dynamenapumila (L). Larval settlement in Dynamena pumila (L). J ExpMar Biol Ecol 208:73–85.
Otto JJ. 1976. Early development and planula movement inHaliclystus (Schyphozoa: Stauromedusae). In: Mackie GO,editor. Coelenterate ecology and behavior. New York:Plenum Press. p 319–329.
Parkefelt L, Ekstrom P. 2009. Prominent system of RFamideimmunoreactive neurons in the rhopalia of box jellyfish(Cnidaria: Cubozoa). J Comp Neurol 516:157–165.
Plickert G. 1989. Proportion-altering factor (PAF) stimulatesnerve-cell formation in Hydractinia echinata. Cell Differ Dev26:19–27.
Plickert G, Schneider B. 2004. Neuropeptides and photicbehavior in Cnidaria. Hydrobiologia 530:49–57.
Plickert G, Kroiher M, Munck A. 1988. Cell-proliferation and earlydifferentiation during embryonic development and metamor-phosis of Hydractinia echinata. Development 103:795–803.
Plickert G, Schetter E, Verhey-Van-Wijk N, Schlossherr J,Steinbuchel M, Gajewski M. 2003. The role of alpha-ami-dated neuropeptides in hydroid development -LWamidesand metamorphosis in Hydractinia echinata. Int J Dev Biol47:439–450.
Piperno G, Fuller MT. 1985. Monoclonal antibodies specificfor an acetylated form of a-tubulin recognize the antigenin cilia and flagella from a variety of organisms. J Cell Biol101:2085–2094.
Raikova OI, Reuter M, Kotikova EA, Gustafsson MKS. 1998. Acommissural brain! The pattern of 5-HT immunoreactivityin Acoela (Plathelminthes). Zoomorphology 118:69–77.
Reynolds ES. 1963. The use of lead citrate at high pH as anelectron-opaque stain in electron microscopy. J Cell Biol17:208–212.
Roosen-Runge EC. 1967. Gastrovascular system of smallhydromedusae: mechanisms of circulation. Science 156:75–76.
Ryan JF, Burton PM, Mazza ME, Kwong GK, Mullikin JC, FinnertyJR. 2006. The cnidarian-bilaterian ancestor possessed atleast 56 homeoboxes: evidence from the starlet sea anem-one, Nematostella vectensis. Genome Biol 7:R64.
Schmich J, Rudolf R, Trepel S, Leitz T. 1998a. Immunohisto-chemical studies of GLWamides in Cnidaria. Cell TissueRes 294:169–177.
Schmich J, Trepel S, Leitz T. 1998b. The role of GLWamidesin metamorphosis of Hydractinia echinata. Dev Genes Evol208:267–273.
Schmidt-Rhaesa A. 2009. Morphology and deep metazoanphylogeny. Zoomorphology 128:199–200.
Schwoerer-Bohning B, Kroiher M, Muller WA. 1990. Signaltransmission and covert prepattern in the metamorphosisof Hydractinia echinata. Dev Genes Evol 198:245–251.
Seipel K, Schmid V. 2005. Evolution of striated muscle: jelly-fish and the origin of triploblasty. Dev Biol 282:14–26.
Siddiqui SS, Aamodt E, Rastinejad F, Culotti J. 1989. Anti-tubulin monoclonal-antibodies that bind to specific neuronsin Caenorhabditis elegans. J Neurosci 9:2963–2972.
Sommer C. 1992. Larval biology and dispersal of Eudendriumracemosum (Hydrozoa, Eudendridee). Sci Mar 56:205–211.
Spring J, Yanze N, Josch C, Middel AM, Winninger B, SchmidV. 2002. Conservation of Brachyury, Mef2, and Snail in themyogenic lineage of jellyfish: a connection to the meso-derm of Bilateria. Dev Biol 244:372–384.
Thomas MB, Edwards NC. 1991. Cnidaria: Hydrozoa. In: Harri-son FW, Westfall JA, editors. Microscopic anatomy ofinvertebrates, vol 2. New York: Wiley-Liss. p 91–183.
Thomas MB, Freeman G, Martin VJ. 1987. The embryonic ori-gin of neurosensory cells and the role of nerve cells inmetamorphosis of Phialidium gregarium. Invert Reprod Dev11:265–287.
Watanabe H, Fujisawa T, Holstein TW. 2009. Cnidarians andthe evolutionary origin of the nervous system. Dev GrowthDiffer 51:167–183.
Werner B. 1984. Stamm Cnidaria, Nesseltiere. In: Gruner HE,editor. Wirbellose Tiere. Stuttgart: Gustav Fischer. p 10–305.
Widersten B. 1968. On the morphology and development insome cnidarian larvae. Zool Bidr Upps 37:139–182.
Yanze N, Spring J, Schmidli C, Schmid V. 2001. Conservationof Hox/ParaHox-related genes in the early development ofa cnidarian. Dev Biol 236:89–98.
Yuan D, Nakanishi N, Jacobs DK, Hartenstein V. 2008. Embry-onic development and metamorphosis of the scyphozoanAurelia. Dev Genes Evol 218:525–539.
Neural complexity in hydrozoan larvae
The Journal of Comparative Neurology | Research in Systems Neuroscience 1951