Cell proliferation is necessary for the regeneration of oral structures in the anthozoan cnidarian Nematostella vectensis
© Passamaneck and Martindale; licensee BioMed Central Ltd. 2012
Received: 5 July 2012
Accepted: 27 November 2012
Published: 4 December 2012
The contribution of cell proliferation to regeneration varies greatly between different metazoan models. Planarians rely on pluripotent neoblasts and amphibian limb regeneration depends upon formation of a proliferative blastema, while regeneration in Hydra can occur in the absence of cell proliferation. Recently, the cnidarian Nematostella vectensis has shown potential as a model for studies of regeneration because of the ability to conduct comparative studies of patterning during embryonic development, asexual reproduction, and regeneration. The present study investigates the pattern of cell proliferation during the regeneration of oral structures and the role of cell proliferation in this process.
In intact polyps, cell proliferation is observed in both ectodermal and endodermal tissues throughout the entire oral-aboral axis, including in the tentacles and physa. Following bisection, there is initially little change in proliferation at the wound site of the aboral fragment, however, beginning 18 to 24 hours after amputation there is a dramatic increase in cell proliferation at the wound site in the aboral fragment. This elevated level of proliferation is maintained throughout the course or regeneration of oral structures, including the tentacles, the mouth, and the pharynx. Treatments with the cell proliferation inhibitors hydroxyurea and nocodazole demonstrate that cell proliferation is indispensable for the regeneration of oral structures. Although inhibition of regeneration by nocodazole was generally irreversible, secondary amputation reinitiates cell proliferation and regeneration.
The study has found that high levels of cell proliferation characterize the regeneration of oral structures in Nematostella, and that this cell proliferation is necessary for the proper progression of regeneration. Thus, while cell proliferation contributes to regeneration of oral structures in both Nematostella and Hydra, Nematostella lacks the ability to undergo the compensatory morphallactic mode of regeneration that characterizes Hydra. Our results are consistent with amputation activating a quiescent population of mitotically competent stem cells in spatial proximity to the wound site, which form the regenerated structures.
Regeneration is mediated by a variety of cell behaviors depending upon the organism. Broadly, the role of cell proliferation in regeneration is generally grouped into two categories: epimorphosis, in which regeneration is mediated by cell proliferation, and morphallaxis, in which regeneration can occur in the absence of cell proliferation. The source of proliferative cells and their differentiation capacity varies among different organisms that display epimorphic regeneration. In planarians, which have become the recent focus of intensive research, regeneration is mediated by neoblasts, pluripotent stem cells which undergo proliferation and subsequent differentiation to replace lost tissues . In the classical system of urodele amphibian regeneration, cell proliferation is also involved, but proliferative cells originate though dedifferentiation of cells . New tissues in the regenerated portion of the limb appear to be derived from the same tissue types in the limb stump, and thus appear to be lineage restricted following an amplification phase . The hydrozoan cnidarian Hydra, the best studied exemplar of morphallaxis, can undergo regeneration of oral structures, such as the mouth and tentacles, when cell proliferation is blocked [4, 5], although recent work has shown that normal regeneration in Hydra is characterized by increased cell proliferation [6, 7]. These examples demonstrate the surprisingly large variation in “regenerative strategies” displayed by different metazoan taxa, and beg the question about the evolution of “stable” cell fates and the molecular basis of cell communication and differentiation.
The anthozoan cnidarian Nematostella vectensis has recently emerged as a basally divergent metazoan system for studies of developmental patterning . Like Hydra, Nematostella is a member of the diploblastic clade Cnidaria, which is a sister group to the Bilateria. However, the two species are distantly related, with Nematostella being a member of the clade Anthozoa, while Hydra is in the clade Hydrozoa. These two clades diverged 600 million years ago, and have likely been evolving independently from one another for longer than have the lineages leading to amphibians and planarians. Nematostella has generated interest for the fact that, unlike most other cnidarians, it can be readily spawned in the laboratory, allowing for experimental comparisons of patterning during the developmental events of embryogenesis, asexual reproduction, and regeneration [8–10].
Although a number of functional studies have begun to detail the patterning mechanisms underlying embryogenesis in Nematostella (e.g. [11–17]), and the genome has been sequenced , the process of regeneration has received comparatively little attention. The present study investigates patterns of cell proliferation during the regeneration of oral structures in Nematostella, and evaluates their role in the formation of regenerated structures.
Morphogenesis during oral regeneration
Cell proliferation in intact polyps
Animals labeled one week after feeding continue to display cell proliferation though the body (Figure 2B, E), although at lower levels than at two days after amputation (Figure 2G). High concentrations of proliferating cells are observed in the oral ring where new tentacles are forming, and at the base of existing elongate tentacles (Figure 2E). Again, proliferating cells are almost completely absent from the distal tips of elongate tentacles (Figure 2E). For all tissues the percentage of EdU labeled cells was significantly lower at one week after feeding than at two days after feeding (p value < 0.05; Figure 2G).
By three weeks after feeding, the percentage of proliferating cells in polyps has decreased dramatically (Figure 2C, F, G). EdU labeled cells are nearly absent from the body column ectoderm and endoderm, including the mesenteries (Figure 2F, G). More cell proliferation is observed in the tentacle ectoderm and pharynx, but here also the proportion of proliferating cells is decreased from one week after feeding (Figure 2F, G). For all tissues the percentage of EdU labeled cells was significantly lower at three weeks after feeding than at one week after feeding (p value < 0.05; Figure 2G)
Cell proliferation during oral regeneration
By 24 hours after amputation there is a marked increase in the percentage of proliferative cells in both the ectoderm and endoderm close to the wound site (Figure 3C, G, Q, R). The percentage of proliferating cells in both the ectoderm and endoderm continues to increase rapidly between 24 hours and 48 hours post amputation (Figure 3Q, R), reaching a maximum at 48 hours after amputation in the ectoderm (Figure 3Q), and between 48 hours and 72 hours post amputation in the endoderm (Figure 3R). Between 24 hours and 36 hours post amputation, proliferative cells are distributed fairly evenly in the tissue near the wound site (Figure 3C, G, D, H). By 48 hours post amputation the majority of proliferating cells in the ectoderm are located in the tentacle buds, while the majority of proliferating cells in the endoderm are located in the reforming pharynx (Figure 3I, M). This distribution of proliferating cells is maintained through 120 hours post amputation (Figure 3J-L, N-P), when regeneration of oral structures is nearly complete and the percentage of proliferating cells in both the endoderm and ectoderm has decreased from its maximum (Figure 3Q, R).
Cell proliferation is required for Nematostellaregeneration
To test the importance of cell proliferation during different periods of the regeneration process, amputated polyps were exposed to pulse treatments of hydroxyurea or nocodazole, washed with 1/3x filtered seawater to remove the inhibitor, and incubated until 96 hours after amputation to determine effects on tentacle growth (Figure 5A). Polyps were also incubated with EdU at 96 hours after amputation to test for the perdurance of effects on cell proliferation after pulse treatments with inhibitors and the re-initiation of cell proliferation. Pulse treatments were performed over three periods: from 2 to 18 hours after amputation, when levels of cell proliferation are similar to those before amputation; from 18 to 30 hours after amputation, when there is a dramatic increase in the levels of proliferating cells; and from 30 to 42 hours after amputation, when the tentacle buds begin to form.
Treatment with hydroxyurea during all three periods produced similar results, with no statistical difference in tentacle lengths between treatments (p value = 0.30, one-way ANOVA; Figure 5D, F-H). In each case the tentacle length at 96 hours after amputation was approximately half that of untreated polyps the same time after amputation (control: 214.3 μm ± 19.7 μm; hydroxyurea 2–18 hpa: 95.3 μm ± 8.7 μm; hydroxyurea 18–30 hpa: 88.0 μm ± 9.5 μm; hydroxyurea 30–42 hpa: 112.2 μm ± 12.2 μm). All three treatments also showed similar levels of cell proliferation, primarily in the tentacles, oral disc, and pharynx (Figure 5J-L). In contrast, in nocodazole treatments tentacle regeneration was only observed in treatments from 2 to 18 hours after amputation (81.9 μm ± 12.0 μm; Figure 5D, N). In both later treatments, from 18 to 30 hours after amputation and 30 to 42 hours after amputation, no tentacle growth was observed by 96 hours (Figure 5D, O, P).
In polyps treated with nocodazole from 2 to 18 hours after amputation, the number of proliferating cells at 96 hours after amputation was comparable to that in all three pulse treatments with hydroxyurea (Figure 5J, K, L, R). In the later treatments, from 18 to 30 hours and 30 to 42 hours, proliferating cells were observed at 96 hours, but the number was greatly reduced (Figure 5S, T). No regeneration of oral structures was observed in these later nocodazole treated polyps after several weeks in 1/3x seawater (data not shown).
Regeneration can be reinitiated in drug treated animals following secondary amputation
Polyps incubated with EdU at 24 hours after amputation showed levels of cell proliferation comparable with those observed in other experiments, described above (Figure 6B, F). However, when polyps were incubated with EdU following nocodazole treatment from 18 to 24 hours after amputation, no detectable cell proliferation was observed (Figure 6C, G). 96 hours after amputation, untreated polyps displayed regeneration of the tentacles (91.5 μm ± 11.8 μm), while nocodazole treated polyps showed no outgrowth of tentacles (Figure 6J, K, N).
Untreated polyps which were bisected a second time showed high levels of cell proliferation at the wound site 24 hours after the second amputation (Figure 6D, H). Polyps bisected a second time following incubation with nocodazole showed comparable levels of cell proliferation 24 hours after the second bisection (Figure 6E, I). Both control and nocodazole treated polyps underwent regeneration after the second amputation, with similar tentacle lengths achieved 96 hours after the second amputation (recut control: 84.0 μm ± 15.0 μm; recut nocodazole treated: 74.8 μm ± 0.5 μm; p value = 0.61; Figure 6L-N).
Nematostella polyps demonstrate the ability to undergo rapid regeneration of oral structures, including the tentacles, mouth, and pharynx after amputation. Initial wound closure is very rapid, beginning almost immediately after bisection of the animal. The finding that muscle fibers recede from the wound site shortly after amputation is consistent with observations of regeneration made in Myosin Heavy Chain1 transgenic polyps by Renfer et al. . Following initial wound closure, relatively little morphological change is seen until the tentacle buds begin to emerge, two to three days later. Following this, the tentacles grow progressively and the mouth and pharynx are reformed.
Cell proliferation in intact polyps
Cell proliferation occurs throughout the polyp, including in the mouth, oral disc, tentacles and physa. The one part of the polyp which appears to be relatively free of proliferating cell is the tentacle tips, which are densely packed with fully differentiated cnidocytes . These results suggest that growth occurs throughout the polyp, rather than at a localized growth zone. This distribution of proliferating cells throughout the polyp is comparable to previous results from another anemone, Aiptasia, where tritiated thymidine uptake was observed along the length of the oral-aboral axis, including in the tentacles . As in Nematostella, cell proliferation in Aiptasia was found to be highest in the tentacles and the oral disc. Singer  reported relatively little labeling with tritiated thymidine in the endoderm of Aiptasia as compared with the ectoderm. Whether this represents a distinct difference in rates of proliferation in the two tissue layers, or is due to a technical limitation of the experiments, is uncertain. Although levels of EdU incorporation in Nematostella were greater in the ectoderm than in the endoderm of the tentacles, levels of incorporation were nearly equivalent in the body column ectoderm and endoderm (including the mesenteries). Cell proliferation in tentacles has also been observed in the scyphozoan Aurelia during metamorphosis of the planula into the primary polyp . This is in contrast with studies of Hydra, where cell proliferation is localized to the body column, and is notably absent from the tentacles, as well as the pedal disc. Likewise, an absence of proliferating cells in the tentacles has also been observed in other hydrozoans, including in the polyps of Hydractinia, Tubularia, and Podocoryne, and in the hydromedusae of Clytia and Podcoryne.
Localized cell proliferation in the body column, and absence from the tentacles, appears to be a common feature within hydrozoans, and may be the ancestral state for the Hydrozoa. Our finding of cell proliferation within the tentacles and physa of Nematostella, along with previous work in Aiptasia, demonstrates that growth in actinarian anthozoans occurs locally throughout the body, rather than through the movement of cells from the body column to the extremities, as is the case in hydrozoans. Additional taxonomic sampling will be necessary to determine the ancestral state for polyp growth in the Cnidaria in general.
Cell proliferation during regeneration of oral structures
We have found that in Nematostella polyps there is a slow increase in the percentage of proliferating ectodermal cells during the initial 20 hours following amputation of the oral structures. During the period from 20 to 24 hours after amputation there is a rapid increase in the percentage of proliferating cells in the ectoderm close to the wound site. This increase in the percentage of proliferating cells reaches a maximum around 48 hours after amputation, and slowly decreases thereafter, as the tentacles, mouth, and pharynx are reformed. In the endoderm, cell proliferation remains at a low level until 16 hours after amputation, and then undergoes a steady increase until at least 48 hours after amputation, before gradually decreasing during the latter morphogenetic period of regeneration. Therefore, the greatest increase in the levels of cell proliferation occur in the period after wound healing and before or during the early stages of oral structure morphogenesis. In Aiptasia, levels of proliferation during regeneration were likewise reported to increase dramatically after the initial period of wound healing . Interestingly, in Aiptasia proliferation was reported to be localized primarily to the ectoderm, with only minimal proliferation observed in the endoderm . In Nematostella, the overall trend in levels of cell proliferation during regeneration is comparable between the ectoderm and endoderm, although a higher maximum level of proliferation is reached in the ectoderm.
Cell proliferation is required for regeneration of oral structures
Pulse-chase experiments with EdU labeling and inhibitor treatment demonstrated that both hydroxyurea and nocodazole were effective in inhibiting cell proliferation, and both compounds were utilized to evaluate the role of cell proliferation during regeneration of the oral structures. Extended incubations from 18 to 96 hours after amputation with either hydroxyurea or nocodazole resulted in no regeneration of the tentacles, mouth, or pharynx, evidencing the requirement of cell proliferation for regeneration of each of these structures. Pulse-chase experiments with inhibitors demonstrated that cell proliferation through the initial 42 hours after amputation appears to contribute to regeneration. With hydroxyurea, comparable reductions in tentacle length at 96 hours after amputation were observed following treatments from 2 to 18 hours after amputation, the period of wound healing, from 18 to 30 hours after amputation, the period of increased proliferation, and from 30 to 42 hours after amputation, the period of initial tentacle bud formation. In each case, the effects of hydroxyurea were reversible, with cell proliferation and regeneration proceeding after removal of the inhibitor. While nocodazole treatment from 2 to 18 hours after amputation likewise reduced tentacle length, treatments from 18 to 30 hours after amputation or from 30 to 42 hours after amputation permanently blocked the progression of regeneration. These results suggest that cell proliferation during the initial wound healing stage contributes to, but is not required for, the progression of regeneration. However, the increased levels of cell proliferation which are observed later are essential for the progression of regeneration. It is uncertain whether the differences in the effects of these two inhibitors may be attributable to their mechanisms of action. Hydroxyurea, which blocks DNA synthesis, has been shown to be reversible in cell culture following removal of the inhibitor [28, 29]. Nocodazole, which blocks mitosis by binding tubulin and preventing microtubule polymerization, has been shown to be reversible in vitro and in cell cultures [30, 31]. However, our results suggest that it permanently blocks proliferation in Nematostella under the conditions used. The relative absence of EdU incorporation following nocodazole treatment suggests that cells at the wound site may undergo multiple rounds of proliferation, which are blocked by exposure to the inhibitor. Experiments conducted during the study to address this question were equivocal (data not shown). Future investigations will be required to determine the precise fate of proliferating cells over the course of regeneration.
We were able to overcome the inhibition of regeneration by nocodazole though secondary amputation. Polyps that were re-amputated following exposure to nocodazole initiated cell proliferation at the new wound site and grew tentacles at rates comparable to polyps in control treatments. These results suggest that initiation of cell proliferation and regeneration may be a localized event linked to wound closure and healing. It appears likely that a distinct population of cells at the secondary wound site were unaffected by the nocodazole treatment and begin to proliferate once stimulated by the secondary amputation. The nature of these cells, whether they are stem cells or dedifferentiated cells that have reentered the cell cycle, remains to be determined. One factor that may be mediating the response to amputation is the canonical Wnt/ß-catenin pathway, as treatments with alsterpaullone, which prevents degradation of cytosolic ß-catenin, have been shown to bias Nematostella regeneration towards oral fates .
The role of cell proliferation in Nematostella appears to be distinct from that in the hydrozoan cnidarian Hydra. Regeneration in Hydra has classically been described as morphallactic, based upon numerous studies have demonstrated the ability of Hydra to undergo reformation of oral structures in the absence of cell proliferation [4, 5, 33–36]. However, in unperturbed animals increased cell proliferation at the wound site has been shown to characterize regeneration response both shortly after amputation in response to Wnt3 signaling from apoptotic cells [7, 37], and in association with neurogenesis 24 to 48 after amputation, prior to the emergence of the tentacle buds [6, 38]. Although regeneration of oral structures can proceed in Hydra in the absence of cell proliferation, a number of abnormalities, including changes in the number of tentacles formed, have been observed in polyps where cell proliferation has been inhibited to produce polyps lacking nerve cells . In Nematostella we have found an absence of any morphallactic response, with cell proliferation being absolutely required for the regeneration of oral structures, including the tentacles, mouth, and pharynx, in the experiments performed. A role for cell proliferation in regeneration has also been suggested in the scyphozoan Aurelia, where hydroxyurea treatment inhibits the reformation of polyps from isolated tentacle fragments . These results suggest that cell proliferation may be a common feature of oral regeneration in the Cnidaria in general, with Hydra having acquired the ability to undergo regeneration through a compensatory morphallactic mode.
The results of this study demonstrate that increased cell proliferation occurs during the regeneration of oral structures in Nematostella, and is necessary for regeneration to proceed. This epimorphic mode of regeneration differs from the morphallactic regeneration potential in Hydra, which can proceed without the contribution of cell proliferation. Future studies will be needed to determine the origin and character of the proliferative cells that participate in Nematostella regeneration.
Regeneration experiments were performed with polyps raised from in vitro fertilized embryos, and fed weekly with freshly hatched Artemia nauplii until they were approximately 5-10 mm in length when relaxed and had eight or ten tentacles. Amputation was performed three weeks after the last feeding by relaxing the polyps with MgCl2 for ten minutes, and bisecting them a scalpel. In all cases the cut was made orthogonally to the oral-aboral axis of the polyp, at a point approximately 0.5 mm aboral of the pharynx. Amputated aboral fragments less than 2.5 mm in length were excluded from experiments as they failed to produce a robust regeneration response. Amputated fragments were washed several times with 1/3x filtered seawater, and maintained at 22°C for all experiments.
Detection of cell proliferation
Proliferating cells were labeled by incubation with the thymidine analog 5-ethynyl-2′-deoxyuridine (EdU), which was subsequently labeled fluorescently with the Click-It EdU Imaging Kit (Invitrogen, Carlsbad, CA, USA) . EdU incubations for immediate fixation were performed with 100 μM of EdU in 1/3 seawater for 30 minutes. Following incubation, polyps were relaxed in MgCl2 for ten minutes prior to fixation. For pulse-chase experiments, polyps were incubated with 10 μM EdU in 1/3x seawater for 30 minutes, washed 3 times with 1/3x seawater, and maintained in 1/3x seawater with 100 μM thymidine until fixation. Fixations were performed with ice-cold 4% paraformaldehyde and 0.2% glutaraldehyde in 1x PBS for two minutes, followed by 4% paraformaldehyde in 1x PBS for one hour. Detection of EdU with Alexa azide fluorophores was performed following the manufacturer’s protocols. Following detection, polyps were washed three times in 1x PBS with 0.1% Triton X-100 (PTx), and subsequently all nuclei were counterstained with Hoechst 33342 (Invitrogen, Carlsbad, CA, USA) at 10 μg/ml in PTx for 2 hours. Polyps were cleared for imaging with a series of glycerol in 1xPBS at concentrations of 20%, 40%, 60% and 80%. Confocal imaging was performed using a Zeiss LSM 710 microscope (Carl Zeiss Microimaging, Inc., Thornwood, NY, USA) with either a 20x/0.8 NA dry objective or a 40×/1.3 NA oil immersion objective.
Measurement of cell proliferation
To determine the percentage of EdU labeled cells in regenerating polyps, counts were performed in the area extending 350 μm from the initial amputation site. Counts were performed on 1.5 μm optical slices, with 3 slices measured and averaged for each polyp. For each slice, ectodermal and endodermal components were distinguished by eye and separate counts performed for the two tissues. Automated cell counts were performed using Volocity 6.0.1 software (PerkinElmer, Inc., Waltham, MA, USA). For each time point, average values were derived from counts on 5 to 10 individuals.
Measurement of tentacle length
Tentacle morphology was determined by labeling filamentous actin in fixed polyps with BODIPY FL phallacidin (Molecular Probes, Eugene, OR, USA), and counterstaining nuclei with Hoechst 33342 (Invitrogen, Carlsbad, CA, USA). Confocal imaging was performed using a Zeiss LSM 710 microscope (Carl Zeiss Microimaging, Inc., Thornwood, NY, USA) with either a 20x/0.8 NA dry objective or a 40x/1.3 NA oil objective. Length of tentacles was determined using Volocity 6.0.1 software (PerkinElmer, Inc., Waltham, MA, USA), measuring from the base of the tentacle, at the level of the oral disc, to the tip. For animals where no tentacle buds could be distinguished, tentacle length was recorded as zero.
Cell proliferation inhibitor treatments
Cell proliferation was blocked with two inhibitors, hydroxyurea (Sigma-Aldrich, St. Louis, MO, USA) and nocodazole (Sigma-Aldrich, St. Louis, MO, USA). Incubations with hydroxyurea were performed at a concentration of 20 mM. Incubations with nocodazole were performed at a concentration of 0.1 μM. For extended incubations, 1/3x seawater with inhibitor was exchanged with freshly diluted inhibitor every 12 hours. For pulse experiments, polyps were washed with 1/3x filtered seawater a minimum of four times after exposure to the inhibitor.
Experimental data is presented as the mean ± standard error from at least three independent experiments. Data was analyzed with Student’s t-test, with the exception of comparisons between three time-series pulse treatments with hydroxyurea, in which case one-way ANOVA was performed. Differences with p value < 0.05 were considered significant.
Days post feeding
Hours post amputation
Hours post secondary amputation
Weeks post feeding.
- Wagner DE, Wang IE, Reddien PW: Clonogenic neoblasts are pluripotent adult stem cells that underlie planarian regeneration. Science. 2011, 332: 811-816. 10.1126/science.1203983.PubMed CentralView ArticleGoogle Scholar
- Hay ED, Fischman DA: Origin of the blastema in regenerating limbs of the newt Triturus viridescens. An autoradiographic study using tritiated thymidine to follow cell proliferation and migration. Dev Biol. 1961, 3: 26-59. 10.1016/0012-1606(61)90009-4.View ArticleGoogle Scholar
- Kragl M, Knapp D, Nacu E, Khattak S, Maden M, Epperlein HH, Tanaka EM: Cells keep a memory of their tissue origin during axolotl limb regeneration. Nature. 2009, 460: 60-65. 10.1038/nature08152.View ArticleGoogle Scholar
- Hicklin J, Wolpert L: Positional information and pattern regulation in hydra: the effect of gamma-radiation. J Embryol Exp Morphol. 1973, 30: 741-752.Google Scholar
- Cummings SG, Bode HR: Head regeneration and polarity reversal in Hydra attenuata can occur in the absence of DNA synthesis. Dev Genes Evol. 1984, 194: 79-86.Google Scholar
- Miljkovic-Licina M, Chera S, Ghila L, Galliot B: Head regeneration in wild-type hydra requires de novo neurogenesis. Development. 2007, 134: 1191-1201. 10.1242/dev.02804.View ArticleGoogle Scholar
- Chera S, Ghila L, Dobretz K, Wenger Y, Bauer C, Buzgariu W, Martinou J-C, Galliot B: Apoptotic cells provide an unexpected source of Wnt3 signaling to drive Hydra head regeneration. Dev Cell. 2009, 17: 279-289. 10.1016/j.devcel.2009.07.014.View ArticleGoogle Scholar
- Darling JA, Reitzel AR, Burton PM, Mazza ME, Ryan JF, Sullivan JC, Finnerty JR: Rising starlet: the starlet sea anemone, Nematostella vectensis. Bioessays. 2005, 27: 211-221. 10.1002/bies.20181.View ArticleGoogle Scholar
- Reitzel AM, Burton PM, Krone C, Finnerty JR: Comparison of developmental trajectories in the starlet sea anemone: Nematostella vectensis embryogenesis, regeneration, and two forms of asexual fission. Invertebr Biol. 2007, 126: 99-112. 10.1111/j.1744-7410.2007.00081.x.View ArticleGoogle Scholar
- Burton PM, Finnerty JR: Conserved and novel gene expression between regeneration and asexual fission in Nematostella vectensis. Dev Genes Evol. 2009, 219: 79-87. 10.1007/s00427-009-0271-2.View ArticleGoogle Scholar
- Wikramanayake AH, Hong M, Lee PN, Pang K, Byrum CA, Bince JM, Xu R, Martindale MQ: An ancient role for nuclear Beta-catenin in the evolution of axial polarity and germ layer segregation. Nature. 2003, 426: 446-450. 10.1038/nature02113.View ArticleGoogle Scholar
- Martindale MQ, Pang K, Finnerty JR: Investigating the origins of triploblasty: “mesodermal” gene expression in a diploblastic animal, the sea anemone Nematostella vectensis (phylum, Cnidaria; class, Anthozoa). Development. 2004, 131: 2463-2474. 10.1242/dev.01119.View ArticleGoogle Scholar
- Magie CR, Daly M, Martindale MQ: Gastrulation in the cnidarian Nematostella vectensis occurs via invagination not ingression. Dev Biol. 2007, 305: 483-497. 10.1016/j.ydbio.2007.02.044.View ArticleGoogle Scholar
- Kraus Y, Fritzenwanker JH, Genikhovich G, Technau U: The blastoporal organiser of a sea anemone. Curr Biol. 2007, 17: R874-R876. 10.1016/j.cub.2007.08.017.View ArticleGoogle Scholar
- Lee P, Kumburegama S, Marlow H, Martindale M, Wikramanayake A: Asymmetric developmental potential along the animal–vegetal axis in the anthozoan cnidarian, Nematostella vectensis, is mediated by Dishevelled. Dev Biol. 2007, 310: 169-186. 10.1016/j.ydbio.2007.05.040.View ArticleGoogle Scholar
- Rentzsch F, Fritzenwanker JH, Scholz CB, Technau U: FGF signalling controls formation of the apical sensory organ in the cnidarian Nematostella vectensis. Development. 2008, 135: 1761-1769. 10.1242/dev.020784.View ArticleGoogle Scholar
- Layden MJ, Boekhout M, Martindale MQ: Nematostella vectensis achaete-scute homolog NvashA regulates embryonic ectodermal neurogenesis and represents an ancient component of the metazoan neural specification pathway. Development. 2012, 139: 1013-1022. 10.1242/dev.073221.PubMed CentralView ArticleGoogle Scholar
- Putnam NH, Srivastava M, Hellsten U, Dirks B, Chapman J, Salamov A, Terry A, Shapiro H, Lindquist E, Kapitonov VV, Jurka J, Genikhovich G, Grigoriev IV, Lucas SM, Steele RE, Finnerty JR, Technau U, Martindale MQ, Rokhsar DS: Sea anemone genome reveals ancestral eumetazoan gene repertoire and genomic organization. Science. 2007, 317: 86-94. 10.1126/science.1139158.View ArticleGoogle Scholar
- Salic A, Mitchison TJ: A chemical method for fast and sensitive detection of DNA synthesis in vivo. Proc Natl Acad Sci. 2008, 105: 2415-2420. 10.1073/pnas.0712168105.PubMed CentralView ArticleGoogle Scholar
- Renfer E, Amon-Hassenzahl A, Steinmetz PRH, Technau U: A muscle-specific transgenic reporter line of the sea anemone, Nematostella vectensis. Proc Natl Acad Sci. 2010, 107: 104-108. 10.1073/pnas.0909148107.PubMed CentralView ArticleGoogle Scholar
- Marlow HQ, Srivastava M, Matus DQ, Rokhsar D, Martindale MQ: Anatomy and development of the nervous system of Nematostella vectensis, an anthozoan cnidarian. Dev Neurobiol. 2009, 69: 235-254. 10.1002/dneu.20698.View ArticleGoogle Scholar
- Singer II: Tentacular and oral-disc regeneration in the sea anemone, Aiptasia diaphana. J Embryol Exp Morphol. 1971, 26: 253-270.Google Scholar
- Yuan D, Nakanishi N, Jacobs DK, Hartenstein V: Embryonic development and metamorphosis of the scyphozoan Aurelia. Dev Genes Evol. 2008, 218: 525-539. 10.1007/s00427-008-0254-8.View ArticleGoogle Scholar
- Plickert G, Kroiher M, Munck A: Cell proliferation and early differentiation during embryonic development and metamorphosis of Hydractinia echinata. Development. 1988, 103: 795-803.Google Scholar
- Campbell RD: Cell proliferation and morphological patterns in the hydroids Tubularia and Hydractinia. J Embryol Exp Morphol. 1967, 17: 607-616.Google Scholar
- Spring J, Yanze N, Middel AM, Stierwald M, Gröger H, Schmid V: The mesoderm specification factor twist in the life cycle of jellyfish. Dev Biol. 2000, 228: 363-375. 10.1006/dbio.2000.9956.View ArticleGoogle Scholar
- Denker E, Manuel M, Leclère L, Le Guyader H, Rabet N: Ordered progression of nematogenesis from stem cells through differentiation stages in the tentacle bulb of Clytia hemisphaerica (Hydrozoa, Cnidaria). Dev Biol. 2008, 315: 99-113. 10.1016/j.ydbio.2007.12.023.View ArticleGoogle Scholar
- Young CW, Hodaas S: Hydroxyurea: inhibitory effect on DNA metabolism. Science. 1964, 146: 1172-1174. 10.1126/science.146.3648.1172.View ArticleGoogle Scholar
- Adams R, Lindsay J: Hydroxyurea; Reversal of inhibition and use as a cell-synchronizing agent. J Biol Chem. 1966, 242: 1314-1317.Google Scholar
- Hoebeke J, Van Nijen G: Interaction of oncodazole (R 17934), a new anti-tumoral drug, with rat brain tubulin. Biochem Biophys Res Commun. 1976, 69: 319-324. 10.1016/0006-291X(76)90524-6.View ArticleGoogle Scholar
- Zieve GW, Turnbull D, Mullins JM, McIntosh JR: Production of large numbers of mitotic mammalian cells by use of the reversible microtubule inhibitor nocodazole. Nocodazole accumulated mitotic cells. Exp Cell Res. 1980, 126: 397-405. 10.1016/0014-4827(80)90279-7.View ArticleGoogle Scholar
- Trevino M, Stefanik DJ, Rodriguez R, Harmon S, Burton PM: Induction of canonical Wnt signaling by alsterpaullone is sufficient for oral tissue fate during regeneration and embryogenesis in Nematostella vectensis. Dev Dyn. 2011, 240: 2673-2679. 10.1002/dvdy.22774.PubMed CentralView ArticleGoogle Scholar
- Bode HR: Head regeneration in Hydra. Dev Dyn. 2003, 226: 225-236. 10.1002/dvdy.10225.View ArticleGoogle Scholar
- Marcum BA, Campbell RD: Development of Hydra lacking nerve and interstitial cells. J Cell Sci. 1978, 29: 17-33.Google Scholar
- Marcum BA, Campbell RD: Developmental roles of epithelial and interstitial cell lineages in Hydra: analysis of chimeras. J Cell Sci. 1978, 32: 233-247.Google Scholar
- Wittlieb J, Khalturin K, Lohmann JU, Anton-Erxleben F, Bosch TCG: Transgenic Hydra allow in vivo tracking of individual stem cells during morphogenesis. Proc Natl Acad Sci USA. 2006, 103: 6208-6211. 10.1073/pnas.0510163103.PubMed CentralView ArticleGoogle Scholar
- Khalturin K, Anton-Erxleben F, Milde S, Plötz C, Wittlieb J, Hemmrich G, Bosch TCG: Transgenic stem cells in Hydra reveal an early evolutionary origin for key elements controlling self-renewal and differentiation. Dev Biol. 2007, 309: 32-44. 10.1016/j.ydbio.2007.06.013.View ArticleGoogle Scholar
- Holstein TW, Hobmayer E, David CN: Pattern of epithelial cell cycling in Hydra. Dev Biol. 1991, 148: 602-611. 10.1016/0012-1606(91)90277-A.View ArticleGoogle Scholar
- Sacks PG, Davis LE: Production of nerveless Hydra attenuata by hydroxyurea treatments. J Cell Sci. 1979, 37: 189-203.Google Scholar
- Lesh-Laurie G, Hujer A, Suchy P: Polyp regeneration from isolated tentacles of Aurelia scyphistomae: a role for gating mechanisms and cell division. Hydrobiologia. 1991, 216: 91-97. 10.1007/BF00026448.View ArticleGoogle Scholar
This article is published under license to BioMed Central Ltd. This is an Open Access article distributed under the terms of the Creative Commons Attribution License (http://creativecommons.org/licenses/by/2.0), which permits unrestricted use, distribution, and reproduction in any medium, provided the original work is properly cited.