Primordial germ cells (PGCs) give rise to gametes that are responsible for the development of a new organism in the next generation. Two modes of germ line specification have been described: the inheritance of asymmetrically-localized maternally provided cytoplasmic determinants and the induction of the PGC fate by other cell types.
PGCs specification in zebrafish appears to depend on inheritance of germ plasm in which several RNA molecules such as vasa and nanos reside. Whether the specification mode of PGCs found in zebrafish is general for other fish species was brought into question upon analysis of olvas expression – the vasa homologue in another teleost, medaka (Oryzias latipes). Here, in contrast to the findings in zebrafish, the PGCs are found in a predictable position relative to a somatic structure, the embryonic shield. This finding, coupled with the fact that vasa mRNA, which is localized to the germ plasm of zebrafish but does not label a similar structure in medaka opened the possibility of fundamentally different mechanisms governing PGC specification in these two fish species.
Results
In this study we addressed the question concerning the mode of PGC specification in medaka using embryological experiments, analysis of RNA stability in the PGCs and electron microscopy observations. Dramatic alterations in the somatic environment, i.e. induction of a secondary axis or mesoderm formation alteration, did not affect the PGC number. Furthermore, the PGCs of medaka are capable of protecting specific RNA molecules from degradation and could therefore exhibit a specific mRNA expression pattern controlled by posttrancriptional mechanisms. Subsequent analysis of 4-cell stage medaka embryos using electron microscopy revealed germ plasm-like structures located at a region corresponding to that of zebrafish germ plasm.
Conclusion
Taken together, these results are consistent with the idea that in medaka the inheritance of maternally provided asymmetrically-localized cytoplasmic determinants directs cells to assume the germ line fate similar to zebrafish PGCs.
Background
Two basic strategies for the specification of primordial germ cells (PGCs) have been described. In Drosophila, C. elegans and Xenopus the inheritance of germ plasm with associated germ cell determinants appears to be required for PGC formation [1–3]. In these organisms, maternally provided asymmetrically-localized germ plasm, or germ plasm-like structures that are visible in electron micrographs (so called "nuage") are found in positions where the PGCs are formed. In Drosophila it has been shown that the germ plasm has an instructive role in directing nuclei to the germline [4] while zebrafish embryos from which the germ plasm was removed lacked germ cells [5]. In mouse (and by extension other mammals) and urodelean amphibians the mechanisms of germline specification are different. Here, morphologically distinct germ plasm has not been identified in early embryos but rather, as revealed in transplantation experiments, cellular interactions are thought to be responsible for PGC specification [6, 7]. Consistently, the formation of the founding population of PGCs in the mouse was shown to depend on extracellular factors of the bone morphogenetic protein (BMP) family [8–11]. Whereas the actual specification and formation of PGCs in mammals and in urodeles appear to be independent of germ plasm, material resembling nuage, a germ plasm organelle, is found in germ cells of these organisms at later developmental stages [12, 13].
Germ-cell specification in fish was studied mainly in bony fish (teleosts) where the work relied on observations using light and electron microscopy. The germ cells were recognized by their large size and by the typical electron dense nuage-like structures. Using these criteria, the earliest time point at which germ cells could be recognized in teleosts was around the onset of somitogenesis [14–16]. Some investigators deduced that the position where the PGCs were first identified was their site of origin (For references see [17]). Transplantation experiments of the embryonic shield, the fish organizer, in the teleost Fundulus, to the extraembryonic yolk sac of hosts resulted in, among other tissues, the development of germ cells and gonads with the highest frequency of germ cells found when the posterior quarter of the Fundulus shield was grafted [18, 19]. One could not exclude the possibility however, that a small population of PGCs existed already before the end of gastrulation and migrated to the position where they were identified either morphologically or by embryological transplantation experiments. Thus, the question of the time and place of germ-cell origin in fish remained open.
The first molecular marker for PGCs in fish is the zebrafish vasa mRNA [20] an ATP-dependent RNA helicase of the DEAD-box family [21, 22] that is expressed in PGCs of many species (reviewed in [23]). vasa was originally identified in Drosophila as a maternal effect gene required for the formation of abdominal segments and for germ-cell specification [24]. Similar to many other organisms, zebrafish vasa mRNA is maternally supplied and it is detected in the PGCs during all stages of germ line development [20, 25–28]. Close examination by whole-mount in situ hybridization at the 2- and 4-cell stages revealed that the vasa transcript is enriched at the marginal positions of the first two cleavage planes leading to the formation of four stripes of intense vasa RNA staining [20, 25] (Fig. 1A). Interestingly, transmission electron microscopy showed that at the 4-cell stage vasa RNA is embedded within an electron dense matrix that resembles nuage, indicating that at this stage the RNA resides within the zebrafish germ plasm [28]. The position of the germ plasm and its early segregation among the first blastomeres strongly support the notion that in zebrafish cells are directed to the germ line fate by the action of determinants present in the germ plasm [28]. Consistently, inhibiting the translation of RNA molecules that are localized to the germ plasm of the zebrafish can result in severe defects in PGC development (e.g. [29, 30]).
Figure 1
The early expression patterns of zebrafish-vasa, medaka-olvas and medaka-nanos1 mRNAs. In zebrafish, the vasa transcript is enriched at the marginal positions of the first two cleavage planes (A), while at a similar stage olvas mRNA is uniformly distributed throughout the cytoplasm of all blastomers (B). Throughout development in zebrafish, the vasa mRNA is expressed exclusively in the PGCs that can be found in random dorsoventral positions during blastula and gastrula stages (arrowheads in C). In contrast, at the first time point when medaka PGCs can be observed (stage 16), they are found on both sides of the embryonic shield on the dorsal side of the embryo (arrows in D). All images shown are whole-mount in situ hybridizations. The probes used are: vasa (A), vasa and chordin (C), olvas (B, D) and nanos1 (E to H). A, B, E and H are animal view, C is a lateral view with the dorsal aspect (labeled with chordin) to the left and D is a dorsal view, F and H are lateral views.
The findings obtained in zebrafish were extended to suggest that generally in fish, PGCs are specified by determinants found in the germ plasm and that the position of the germ plasm could be inferred from the position of RNA molecules such as vasa and nanos which mark the early germ plasm. Surprisingly, the cloning of the vasa and nanos genes from another teleost, medaka (Oryzias latipes) and analysis of their mRNA expression patterns did not provide direct support for the notion that germ plasm is responsible for PGC specification in all fish species [31, 32]. In contrast to the enrichment of vasa transcripts in the position of the germ plasm observed in zebrafish, the transcripts of olvas, the medaka vasa homologue, were uniformly distributed until stage 16 at late gastrulation ([31], Fig. 1B and 1D). At this stage, PGCs, recognized by higher levels of olvas expression, are found on either side of the shield, the fish organizer [31]. Similarly, medaka nanos transcripts did not aggregate at the two first cleavage planes (Fig. 1E to 1H). As mentioned above, in zebrafish the germ plasm contains vasa and nanos mRNAs and is found at the distal parts of the first two cleavage planes. These four locations are randomly oriented relative to the dorsal aspect of the embryo leading to specification of PGCs in random dorsoventral positions [26]. In contrast, at these stages, olvas and nanos mRNAs were found to be uniformly distributed in the corresponding stages and when the PGCs are first observed using olvas as a molecular marker, they are found in a defined position relative to somatic structures. If the early expression site of vasa and its homologues indeed mark the site and stage of PGC origin, then the expression pattern of olvas would imply a different mechanism for specifying PGC in medaka.
In this work we investigate the question of the mechanisms responsible for PGC specification in medaka. We determine the effect of perturbations in somatic development on PGC specification and describe the properties of medaka PGCs regarding the metabolism of specific RNA molecules. The results presented here are consistent with the notion that despite the differences in the expression pattern of vasa during early embryogenesis in these two teleosts that represent totally different branches of the phylogenetic tree, it is likely that similar basic mechanisms are responsible for PGC specification.
Results and Discussion
Several lines of evidence strongly indicate that in mouse the PGC fate is induced by signals that originate in adjacent tissues. In this organism, germ cells arise just before or during early gastrulation, around the proximal part of the epiblast adjacent to extra-embryonic tissues [6–11]. The finding that medaka PGCs are first detected at a specific position relative to the embryonic shield ([31] and Fig. 1D) could be interpreted as evidence for induction of PGCs by the adjacent somatic cells. Consistent with this suggestion, axial mesodermal tissues in fish are known to be capable of inducing cell fate in adjacent tissues (e.g. [33]).
Medaka PGCs number is independent of patterning of somatic tissues
If PGCs in medaka are induced through interactions with somatic tissues at the site where they are first observed, then specific alterations in the development of these tissues are expected to bring about changes in the position and number of PGCs. To address this point early somatic development was affected in two ways: either by injecting b-catenin thereby generating two embryonic axes in a single embryo (Fig. 2A,B and 2C), or by disturbing early axial mesoderm specification through BMP pathway modulation (Fig. 2D to 2P).
Figure 2
The effect of axis duplication and mesoderm induction modulation in medaka on PGC number. (A, B and C) Induction of a complete secondary embryonic axis was achieved by injection of β-catenin at the 8- and 16-cell stage. The injected embryos were fixed at stages 17 and 23 and their PGCs visualized by in situ hybridization using an olvas antisense RNA probe. A: a stage 23 control embryo injected with GFP-globin; B: a stage 23 embryo with a duplicated embryonic axis. In both stages analyzed, the average PGC number in embryos with a duplicated axis is similar to that of control embryos (C). (D to P) BMP-mediated mesoderm induction modulation was achieved by injection of either BMP2 (H to K) or dominant negative form of BMP2/4RI (DN(BMP2/4RI)) (L to O). To confirm mesoderm formation alteration, in situ hybridization was performed with either Goosecoid (Gsc) ventrolateral mesodermal marker (F, J and N) or HNF3-b axial mesodermal marker (G, K and O). One day post fertilization (dpf), the average PGC number in embryos with altered mesoderm is similar to that of control embryos (P). The number of embryos analyzed is provided within the corresponding bars.
The first manipulation was carried out by injection of 600 pg β-catenin RNA into one marginal blastomere at the 8- or 16-cell stage (based on the protocol for zebrafish by [34]). This resulted in formation of a complete secondary axis in about 3% of the injected embryos. Control embryos were injected with the same amount of GFP-globin RNA. The injected embryos were fixed at stages 17 and 23 and whole-mount in situ hybridization was performed using an olvas antisense RNA probe to visualize the PGCs (for stage 23 see Fig. 2A and 2B). The position of PGCs in embryos with an induced secondary embryonic axis was similar to that observed in control embryos of the same developmental stage. If PGC fates are indeed induced by somatic tissues of the organizer, one would expect an increase in PGC number when two shields are present in the embryo. However, the average number of PGCs in embryos with duplicated axes was found to be similar to the number of PGCs in control embryos (Fig. 2C).
Mesoderm patterning during early gastrulation was modulated by either overexpressing BMP2 (Fig. 2H to 2K) or expressing a dominant negative form of BMP2/4 receptor I (DN(BMP2/4RI)) (Fig. 2L to 2O), which results in ventralization and dorsalization of mesoderm, respectively. Again, no alteration in the total number of PGCs was observed, although their localization was severely impaired (Fig. 2D to 2P). Thus, the number of PGCs is independent of mesoderm patterning.
These findings do not support the idea that PGC fate is induced by neighboring cells at the site where they are first detected. Rather, these results are more consistent with the model according to which PGCs in medaka are specified by inheritance of pre-localized maternal components whose amount is the limiting factor determining the number of PGCs. As BMP-induced mesoderm formation occurs during gastrulation and the induction of the secondary axis by β-catenin arises at a very early stage of development well before gastrulation initiates, we consider it unlikely that the PGCs are specified by an earlier inductive process.
Medaka PGCs selectively stabilize maternally provided transcripts
As mentioned above, in Drosophila and C. elegans the PGCs are specified by inheritance of maternally provided asymmetrically-localized cytoplasmic determinants. In these organisms, maternally provided transcripts that are expressed in the PGCs are selectively stabilized within these cells while being degraded in somatic cells [35, 36]. Similarly, in zebrafish the mRNA of the vasa gene [37], as well as nanos1 (nos1) mRNA [29, 38] are degraded in somatic cells but are stabilized and translated in cells that contain germ plasm.
If specification of PGCs in medaka occurs by inheritance of germ plasm similar to zebrafish, then the phenomena of differential stability of RNAs between somatic and primordial germ cells is expected to take place in this species, as well.
To examine this point, mRNAs from three zebrafish GFP-fusion constructs, vasa-GFP, GFP-zfvasa 3'UTR and GFP-nos1 3'UTR, were injected into 1- to 2-cell stage medaka embryos. Following the injection of 100 pg RNA, in situ hybridization using an antisense GFP-RNA probe was performed at different times of development to reveal the spatial distribution of the injected fusion RNAs. As a control, RNA encoding GFP flanked by the Xenopus laevis-globin 5' and 3'UTRs was injected and the distribution of this RNA was similarly followed at different stages of development. Remarkably, the zebrafish vasa-GFP-fusion RNA undergoes rapid degradation in the soma and is stabilized in the germ line cells (arrows in Fig. 3D). An analogous distribution is observed for GFP-nos1 3'UTR RNA injected into medaka embryos (data not shown). Interestingly, the results resemble those obtained in zebrafish in several ways: 1. These injected GFP-tagged RNA molecules do not aggregate at the cleavage planes (data not shown). 2. The injected RNA molecules exhibit differential stability between somatic and primordial germ cells. Whereas at the onset of somitogenesis the soma is stained strongly with the antisense GFP probe (Fig. 3B), at stage 23 (12 somites) virtually only the PGCs retain the injected vasa-GFP-fusion RNA (Fig. 3D). In contrast, control embryos show no specific stabilization of the GFP-globin RNA in the germ line but instead, exhibit general RNA degradation in all cells (Fig. 3A and 3C). Consistent with the notion that as in zebrafish, post transcriptional events control differential gene expression between germ cells and somatic cells in other fish species as well, uniform introduction (by injection) of GFP- nos1 3'UTR RNA into 1-cell embryos of Oryzias latipes [see Additional file 2], O. curvinotus [see Additional file 3], O. luzonensis [see Additional file 4] or Betta splendens [see Additional file 5] resulted in germ cells specific GFP expression [see Additional file 1]. Therefore, differential (nos1 3'UTR)-induced post-transcriptional events between somatic and germ cells appears to be a mechanism conserved in different fish lineages representing distantly related branches of the phylogenetic tree (Cypriniformes, Perciformes and Beloniformes).
Figure 3
Stabilization of zebrafish vasa and translational regulation of medaka olvas mRNA in PGCs of medaka. 100 pg of GFP tagged fusion RNAs were injected at the 2-cell stage. (A to D) The embryos were fixed at early somitogenesis and at 12-somite stage and in situ hybridization using a GFP antisense RNA probe was performed to reveal the spatial distribution of the injected RNAs. In the control embryos the GFP-globin RNA is degraded uniformly in all cells (A and C) whereas in vasa-GFP injected embryos (B and D), the PGCs retain the injected RNA (arrows in D) while it is degrading in somatic cells. (E to S) olvas-GFP (E to I) as well as GFP-zfvasa 3'UTR (J to N) constructs were injected in medaka and followed for GFP expression and compared to control GFP-β globin 3'UTR injected embryos (O to S). Interestingly, in medaka, olvas-GFP protein expression was rapidly restricted to PGCs (E to I), while zebrafish vasa 3'UTR did not induced selective GFP expression.
To determine whether this mechanism is relevant for the observed olvas mRNA and protein distributions, a reciprocal experiment was performed in which the original full-length olvas RNA was injected in zebrafish embryos. The analysis of its fate with an antisense olvas probe revealed no specific stabilization of olvas RNA in the PGCs of zebrafish (data not shown). Thus, neither medaka olvas 3'UTR nor olvas open reading frame (ORF) mediate germ cell specific RNA stability in zebrafish. Interestingly, in medaka, olvas-GFP protein expression was rapidly restricted to PGCs (Fig. 3E to 3I), although the olvas-GFP fusion RNA itself was not efficiently differentially stabilized in the PGCs of medaka (data not shown). Therefore, the preferential localization of the olvas-GFP protein to the PGCs (Fig. 3E to 3I) could be attributed to complementary specific posttranscriptional mechanisms: (i) in agreement with Kurokawa et al., a PGC-specific enhanced translation due to the olvas 3'UTR [32]. (ii) Somatic inhibition of translation due to the open reading frame itself. (iii) Soma-specific destabilization of the protein [37].
In addition, like olvas 3'UTR in medaka, zebrafish vasa 3'UTR has been shown to be essential for proper protein PGC localization in zebrafish. Hence, when injected in medaka, GFP-zfvasa 3'UTR failure of selective GFP expression (Fig. 3J to 3N compared to Fig. 3E to 3I and 3O to 3S) points out possible specie-variability of either targeted cis-acting RNA sequence elements or RNA-interacting protein sequence, but likely using a similar conserved mechanism.
Thus, while we provide evidence for the existence of conserved mechanisms governing PGCs specification in zebrafish and medaka, the similarities apparently can not be extended to the control of PGC-specific expression of every molecule, as shown here for the zf-vasa and olvas RNAs. Hence, the mechanisms directing PGC-specific expression of olvas could depend on combined machineries associating enhanced/repressed specific soma/germline translation, protein stabilization and possibly, to a lower extend, RNA stability.
Identification of germ plasm like structures in early Medaka embryos
As the results presented above are consistent with the idea that in medaka, like in zebrafish, inheritance of germ plasm is responsible for the formation of PGCs, we sought to identify germ plasm in early medaka embryos. Both in birds and fish the detection of germ plasm in early embryos was possible only after molecular markers for this organelle became available (the Vasa protein and mRNA respectively) [28, 39]. In the absence of such a molecular marker for the medaka germ plasm we concentrated our efforts on positions equivalent to those where zebrafish germ plasm is found. In zebrafish, the germ plasm with its characteristic electron dense appearance was found to be concentrated below the first two cleavage furrows in 4-cell stage embryos [28]. In medaka, the first 4 blastomeres are much smaller in size and the cleavage furrows are not as pronounced as they are in zebrafish (compare Fig. 4A and 4B). However, within the cytoplasm at the areas where the 4 cells are in contact, distinct electron-dense structures were identified. These structures are formed of amorphous inclusions with a granular fine structure, lacking a surrounding membrane (Fig. 4D and 4F). Serial sections show that this is a rod-like structure approximately 0.5 μm in diameter. These features of the structure correspond to descriptions of germ plasm in many species [40]. The fact that this structure is found exclusively beneath the cleavage furrows, similar to the germ plasm in zebrafish at the corresponding stage leads us to suggest that the observed electron-dense material represents the germ plasm of medaka.
Figure 4
Sections of early 4-cell stage zebrafish and medaka embryos. Semi-thin section of zebrafish (A) and medaka (B) embryos visualized in a light microscope. Arrows indicate the areas shown in C-F representing the cleavage positions. The insets represent the orientation of the sections. Low magnification at the electron microscope showing the region of the germ plasm of zebrafish (C), and the corresponding position in medaka (D). At a higher magnification, the germ plasm of zebrafish is visible as distinct amorphous inclusions with a regular spherical shape and a filamentous fine structure lacking a surrounding membrane (E). At this magnification germ plasm resembling structure composed of irregularly shaped amorphous inclusions with a granular fine structure can be observed in medaka embryos. As described for zebrafish [28], the putative germ plasm of medaka can be followed in serial sections.
Conclusion
Our findings in medaka are consistent with the suggestion that the mode of PGC specification is conserved with zebrafish and possibly other teleosts. First, we show that dramatic alterations in somatic development (axis duplication and mesoderm formation alteration) do not alter the PGC number in medaka, which appears inconsistent with an inductive mode of PGC specification that depend on signals from somatic cells. Second, the process of germ-line specific RNA stabilization shown here for medaka has been described for those organisms whose PGCs are specified by inheritance of maternally provided cytoplasmic determinants. Consistently, material resembling germ plasm was identified in 4-cell stage medaka embryos. The apparent paradox that the vasa-homologue of medaka differs from its zebrafish counterpart with respect to its early spatial distribution and its ability to be subjected to the "degradation-protection" control mechanism may be reconciled by the finding that vasa mRNA appears to be dispensable for early PGC development in zebrafish [41].
Methods
Synthesis of RNA for Embryo Injections
β-catenin sense RNA was transcribed from pT7Ts [34], which contains the full-length zebrafish β-catenin cDNA. The injection of the zebrafish 600 pg β-catenin RNA into one of the marginal blastomeres of 8- and 16-cell stage medaka embryos induced complete secondary axis in 3% of the embryos. As a control, embryos were injected with 600 pg of GFP-globin RNA.
Zebrafish BMP2b and dominant negative truncated version of BMP2/4 receptor I (DN(BMP2/4RI)) were transcribed from pSP64TS and pSP64T respectively. Capped synthetic mRNA were injected (1 nL) into the cytoplasm of a single-cell Medaka embryo at different concentrations (2 to 50 ng/μL and 40 to 200 ng/μL for BMP2b and DN(BMP2/4RI) respectively).
The vasa-GFP construct includes the zebrafish full-length vasa cDNA into which the mmGFP5 [42] open reading frame (ORF) was inserted [37].
The GFP-nos1 3'UTR construct includes the mmGFP5 ORF cloned upstream of the 3'UTR of the zebrafish nanos1 gene [29]. The GFP-zfvasa 3'UTR construct was made by inserting the PCR amplified zebrafish vasa 3'UTR after GFP (XhoI crated site).
The olvas-GFP construct was prepared by inserting the mmGFP5 ORF into the SacII site in the full-length olvas cDNA (obtained from the cab-wild-type strain using the forward oligo AAAAAGCTTTCAGTTTGAAGCTAACAGCAGCAC and reverse oligo AAATCTAGATTTGKTGAAAACTTTTAATTATYAGGAGAA.
GFP-globin: mmGFP5 was cloned in between the globin 5'UTR and globin 3'UTR of pSP64T [37].
All RNA molecules were synthesized using the mMessage mMachinekit (Ambion).
In situHybridization
RNA whole-mount in situ hybridization using olvas [31], nanos [32]goosecoid (Gsc) or HNF3-b DIG labeled probes were performed as previously described for zebrafish [26].
Electron Microscopy
For transmission electron microscopy individual eggs were fixed by immersion in a solution containing 4% paraformaldehyde and 0.1% glutaraldehyde in 0.1 M phosphate buffer at pH 7.4 for 4 h. The chorion was subsequently removed and the eggs were fixed further overnight at 4°C using 2% glutaraldeahyde in 0.1 M phosphate buffer at pH 7.4. After an additional fixation with 1% OsO4 and pre-embedding staining with 1% uranyl acetate, eggs were dehydrated and embedded in EMbed 812 resin (Plano).
The sectioning was performed using a Leica Ultracut ultramicrotome. 600 nm thick sections were stained with tolouidine blue and visualized in a Zeiss light microscope to select the area of interest. Thereafter, 60 nm thick sections were collected and counterstained with 1% uranyl acetate and lead citrate and examined using a Philips CM 120 BioTwin (Philips Inc.Eindhoven, The Netherlands) transmission electron microscope.
Fish Maintenance and Staging
Medaka (Oryzias latipes) wild-type strain cab was maintained as described previously for zebrafish [43]. Developmental stages were determined according the criteria set out by [44].
Declarations
Acknowledgements
We thank S. Schories for Betta splendens embryos, and J. Wittbrodt and F. Loosli and M. Tanaka for the medaka strains and medaka nanos probe, help and encouragement. We thank M. Köprunner and M. Reichman for helpful comments on the manuscript. This work was supported by a grant of the Rudolf-Virchow-Zentrum for Experimental Medicine (DFG Forschungszentrum) to M.S.
Authors’ Affiliations
(1)
Department of Physiological Chemistry I, University of Wuerzburg
(2)
Department of Germ Cell Development, Max-Planck-Institute for Biophysical Chemistry
(3)
Department of Neurobiology, Max-Planck-Institute for Biophysical Chemistry
(4)
Germ Cell Development, Max-Planck-Institute for Biophysical Chemistry, Göttingen and Institute of Cell Biology, ZMBE, University of Münster
(5)
Rudolf-Virchow Center for Experimental Medicine, University of Wuerzburg
References
Rongo C, Broihier HT, Moore L, Van Doren M, Forbes A, Lehmann R: Germ plasm assembly and germ cell migration in Drosophila. Cold Spring Harb Symp Quant Biol. 1997, 62: 1-11.View ArticlePubMedGoogle Scholar
Seydoux G, Strome S: Launching the germline in Caenorhabditis elegans: regulation of gene expression in early germ cells. Development. 1999, 126: 3275-3283.PubMedGoogle Scholar
Houston DW, King ML: Germ plasm and molecular determinants of germ cell fate. Curr Top Dev Biol. 2000, 50: 155-181.View ArticlePubMedGoogle Scholar
Illmensee K, Mahowald AP: Transplantation of posterior polar plasm in Drosophila. Induction of germ cells at the anterior pole of the egg. Proc Natl Acad Sci U S A. 1974, 71: 1016-1020.PubMed CentralView ArticlePubMedGoogle Scholar
Hashimoto Y, Maegawa S, Nagai T, Yamaha E, Suzuki H, Yasuda K, Inoue K: Localized maternal factors are required for zebrafish germ cell formation. Dev Biol. 2004, 268: 152-161.View ArticlePubMedGoogle Scholar
Nieuwkoop PD: The formation of mesoderm in Urodelean amphibians. I. Induction by the endoderm. Wilhelm Roux' Arch EntwMech Org. 1969, 162: 341-373.View ArticleGoogle Scholar
Tam PP, Zhou SX: The allocation of epiblast cells to ectodermal and germ-line lineages is influenced by the position of the cells in the gastrulating mouse embryo. Dev Biol. 1996, 178: 124-132.View ArticlePubMedGoogle Scholar
Lawson KA, Dunn NR, Roelen BA, Zeinstra LM, Davis AM, Wright CV, Korving JP, Hogan BL: Bmp4 is required for the generation of primordial germ cells in the mouse embryo. Genes Dev. 1999, 13: 424-436.PubMed CentralView ArticlePubMedGoogle Scholar
Tsang TE, Khoo PL, Jamieson RV, Zhou SX, Ang SL, Behringer R, Tam PP: The allocation and differentiation of mouse primordial germ cells. Int J Dev Biol. 2001, 45: 549-555.PubMedGoogle Scholar
Ying Y, Qi X, Zhao GQ: Induction of primordial germ cells from murine epiblasts by synergistic action of BMP4 and BMP8B signaling pathways. Proc Natl Acad Sci U S A. 2001, 98: 7858-7862.PubMed CentralView ArticlePubMedGoogle Scholar
Ying Y, Zhao GQ: Cooperation of endoderm-derived BMP2 and extraembryonic ectoderm-derived BMP4 in primordial germ cell generation in the mouse. Dev Biol. 2001, 232: 484-492.View ArticlePubMedGoogle Scholar
Eddy EM: Fine structural observations on the form and distribution of nuage in germ cells of the rat. Anat Rec. 1974, 178: 731-757.View ArticlePubMedGoogle Scholar
Ikenishi KN: Location and ultrastructure of primordial germ cells (PGCs) in Ambystoma mexicanum. Develop Growth Differ. 1978, 20: 1-9.View ArticleGoogle Scholar
Timmermans L, Taverne N: Segregation of primordial germ cells: their numbers ans fate during early development of Barbus conchonius (Cyprinidae, Teleosti) as indicated by 3H-thymidine incorporation. J Morphol. 1989, 202: 225-237.View ArticleGoogle Scholar
Hamaguchi S: A light- and electron-microscopic study on the migration of primordial germ cells in the teleost, Oryzias latipes. Cell Tissue Res. 1982, 227: 139-151.View ArticlePubMedGoogle Scholar
Gevers P, Dulos J, Schipper H, Timmermans LP: Origin of primordial germ cells, as characterized by the presence of nuage, in embryos of the teleost fish Barbus conchonius. Eur J Morphol. 1992, 30: 195-204.PubMedGoogle Scholar
Nieuwkoop PD, Satasurya LA: Primordial germ cell in the chordates. 1979, Cambridge University PressGoogle Scholar
Oppenheimer JM: Extraembryonic transplantation of sections of the fundulus embryonic shield. J Exp Zool. 1959, 140: 247-267.View ArticlePubMedGoogle Scholar
Oppenheimer JM: Extraembryonic transplantation of fragmented shield grafts in Fundulus. J Exp Zool. 1959, 142: 441-459.View ArticlePubMedGoogle Scholar
Yoon C, Kawakami K, Hopkins N: Zebrafish vasa homologue RNA is localized to the cleavage planes of 2- and 4-cell-stage embryos and is expressed in the primordial germ cells. Development. 1997, 124: 3157-3165.PubMedGoogle Scholar
Hay B, Jan LY, Jan YN: A protein component of Drosophila polar granules is encoded by vasa and has extensive sequence similarity to ATP-dependent helicases. Cell. 1988, 55: 577-587.View ArticlePubMedGoogle Scholar
Lasko PF, Ashburner M: The product of the Drosophila gene vasa is very similar to eukaryotic initiation factor-4A. Nature. 1988, 335: 611-617.View ArticlePubMedGoogle Scholar
Schupbach T, Wieschaus E: Maternal effect mutations altering the anterior-posterior pattern of the Drosophila embryo. Roux's Arch Dev Biol. 1986, 195: 302-317.View ArticleGoogle Scholar
Braat AK, Zandbergen T, van de Water S, Goos HJ, Zivkovic D: Characterization of zebrafish primordial germ cells: morphology and early distribution of vasa RNA. Dev Dyn. 1999, 216: 153-167.View ArticlePubMedGoogle Scholar
Weidinger G, Wolke U, Koprunner M, Klinger M, Raz E: Identification of tissues and patterning events required for distinct steps in early migration of zebrafish primordial germ cells. Development. 1999, 126: 5295-5307.PubMedGoogle Scholar
Braat AK, van de Water S, Goos H, Bogerd J, Zivkovic D: Vasa protein expression and localization in the zebrafish. Mech Dev. 2000, 95: 271-274.View ArticlePubMedGoogle Scholar
Knaut H, Pelegri F, Bohmann K, Schwarz H, Nusslein-Volhard C: Zebrafish vasa RNA but not its protein is a component of the germ plasm and segregates asymmetrically before germline specification. J Cell Biol. 2000, 149: 875-888.PubMed CentralView ArticlePubMedGoogle Scholar
Koprunner M, Thisse C, Thisse B, Raz E: A zebrafish nanos-related gene is essential for the development of primordial germ cells. Genes Dev. 2001, 15: 2877-2885.PubMed CentralPubMedGoogle Scholar
Weidinger G, Stebler J, Slanchev K, Dumstrei K, Wise C, Lovell-Badge R, Thisse C, Thisse B, Raz E: dead end, a novel vertebrate germ plasm component, is required for zebrafish primordial germ cell migration and survival. Curr Biol. 2003, 13: 1429-1434.View ArticlePubMedGoogle Scholar
Shinomiya A, Tanaka M, Kobayashi T, Nagahama Y, Hamaguchi S: The vasa-like gene, olvas, identifies the migration path of primordial germ cells during embryonic body formation stage in the medaka, Oryzias latipes. Dev Growth Differ. 2000, 42: 317-326.View ArticlePubMedGoogle Scholar
Kurokawa H, Aoki Y, Nakamura S, Ebe Y, Kobayashi D, Tanaka M: Time-lapse analysis reveals different modes of primordial germ cell migration in the medaka Oryzias latipes. Dev Growth Differ. 2006, 48: 209-221.View ArticlePubMedGoogle Scholar
Blagden CS, Currie PD, Ingham PW, Hughes SM: Notochord induction of zebrafish slow muscle mediated by Sonic hedgehog. Genes Dev. 1997, 11: 2163-2175.PubMed CentralView ArticlePubMedGoogle Scholar
Kelly GM, Erezyilmaz DF, Moon RT: Induction of a secondary embryonic axis in zebrafish occurs following the overexpression of beta-catenin. Mech Dev. 1995, 53: 261-273.View ArticlePubMedGoogle Scholar
Seydoux G, Fire A: Soma-germline asymmetry in the distributions of embryonic RNAs in Caenorhabditis elegans. Development. 1994, 120: 2823-2834.PubMedGoogle Scholar
Bashirullah A, Halsell SR, Cooperstock RL, Kloc M, Karaiskakis A, Fisher WW, Fu W, Hamilton JK, Etkin LD, Lipshitz HD: Joint action of two RNA degradation pathways controls the timing of maternal transcript elimination at the midblastula transition in Drosophila melanogaster. Embo J. 1999, 18: 2610-2620.PubMed CentralView ArticlePubMedGoogle Scholar
Wolke U, Weidinger G, Koprunner M, Raz E: Multiple levels of posttranscriptional control lead to germ line-specific gene expression in the zebrafish. Curr Biol. 2002, 12: 289-294.View ArticlePubMedGoogle Scholar
Mishima Y, Giraldez AJ, Takeda Y, Fujiwara T, Sakamoto H, Schier AF, Inoue K: Differential Regulation of Germline mRNAs in Soma and Germ Cells by Zebrafish miR-430. Curr Biol. 2006, 16: 2135-2142.PubMed CentralView ArticlePubMedGoogle Scholar
Tsunekawa N, Naito M, Sakai Y, Nishida T, Noce T: Isolation of chicken vasa homolog gene and tracing the origin of primordial germ cells. Development. 2000, 127: 2741-2750.PubMedGoogle Scholar
Eddy EM: Germ plasm and the differentiation of the germ cell line. Int Rev Cytol. 1975, 43: 229-280.View ArticlePubMedGoogle Scholar
Braat AK, van de Water S, Korving J, Zivkovic D: A zebrafish vasa morphant abolishes vasa protein but does not affect the establishment of the germline. Genesis. 2001, 30: 183-185.View ArticlePubMedGoogle Scholar
Siemering KR, Golbik R, Sever R, Haseloff J: Mutations that suppress the thermosensitivity of green fluorescent protein. Curr Biol. 1996, 6: 1653-1663.View ArticlePubMedGoogle Scholar
Westerfield M: The zebrafish book. 1995, Oregon: University of Oregon Press.Google Scholar
Iwamatsu T: Stages of normal development in the medaka Oryzias latipes. Mech Dev. 2004, 121: 605-618.View ArticlePubMedGoogle Scholar
Tanaka M, Kinoshita M, Kobayashi D, Nagahama Y: Establishment of medaka (Oryzias latipes) transgenic lines with the expression of green fluorescent protein fluorescence exclusively in germ cells: a useful model to monitor germ cells in a live vertebrate. Proc Natl Acad Sci U S A. 2001, 98: 2544-2549.PubMed CentralView ArticlePubMedGoogle Scholar
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