Advertisement
Research Report
Retinoic acid-driven Hox1 is required in the epidermis for forming the otic/atrial placodes during ascidian metamorphosis
Yasunori Sasakura, Miyuki Kanda, Taku Ikeda, Takeo Horie, Narudo Kawai, Yosuke Ogura, Reiko Yoshida, Akiko Hozumi, Nori Satoh, Shigeki Fujiwara
Development 2012 139: 2156-2160; doi: 10.1242/dev.080234

Summary

Retinoic acid (RA)-mediated expression of the homeobox gene Hox1 is a hallmark of the chordate central nervous system (CNS). It has been suggested that the RA-Hox1 network also functions in the epidermal ectoderm of chordates. Here, we show that in the urochordate ascidian Ciona intestinalis, RA-Hox1 in the epidermal ectoderm is necessary for formation of the atrial siphon placode (ASP), a structure homologous to the vertebrate otic placode. Loss of Hox1 function resulted in loss of the ASP, which could be rescued by expressing Hox1 in the epidermis. As previous studies showed that RA directly upregulates Hox1 in the epidermis of Ciona larvae, we also examined the role of RA in ASP formation. We showed that abolishment of RA resulted in loss of the ASP, which could be rescued by forced expression of Hox1 in the epidermis. Our results suggest that RA-Hox1 in the epidermal ectoderm played a key role in the acquisition of the otic placode during chordate evolution.

INTRODUCTION

Hox1 plays a key role in anterior-posterior axis specification of the CNS in chordates (McGinnis and Krumlauf, 1992), and its expression is regulated by retinoic acid (RA) (Gavalas and Krumlauf, 2000). It has been suggested that this RA-Hox1 network functions in the general ectoderm of chordates (Holland, 2005), which gives rise to both the epidermis and the nervous system. Indeed, in extant cephalochordates and urochordates, RA-mediated Hox1 regulation is observed in the epidermis in addition to the CNS (Schubert et al., 2004; Ikuta et al., 2004; Kanda et al., 2009). In vertebrates, RA-Hox1 is necessary for formation of the otic placode (Hans and Westerfield, 2007; Makki and Capecchi, 2010), a chordate-specific structure in the cranial epidermal ectoderm (Shimeld and Holland, 2000). Because the RA-Hox1 network is crucial for specification of the CNS (Mark et al., 1993), which sends inductive signals to the overlying otic placode, the role of this network in otic placode development has generally been thought to be indirect. However, a recent study has indicated that mouse Hoxa1 is expressed in the otic epithelium (Makki and Capecchi, 2010). Thus, it is possible that the epidermal RA-Hox1 network contributed to the evolutionary innovation of the otic placode in higher chordates; however, the relationship between the epidermal RA-Hox1 network and the otic placode remains unclear.

Here, we report the epidermal functions of the RA-Hox1 cascade in the urochordate Ciona intestinalis. RA-Hox1-deficient animals do not form an atrial siphon placode (ASP), which is homologous to the vertebrate otic placode (Kourakis and Smith, 2007). Tissue-specific expression analysis of Hox1 showed that the RA-Hox1 cascade primarily functions in the epidermis to form the ASP. This study raises the possibility that RA-Hox1 in the epidermal ectoderm played a key role in the acquisition of the otic placode during chordate evolution.

MATERIALS AND METHODS

Transgenic lines

An enhancer detection line EJ[MiTSAdTPOG]124 was created using the jump-starter method (Sasakura et al., 2008). Tg[MiTSAdTPOG]8 (Awazu et al., 2007) was used as a transposon donor. The Minos insertion site of EJ[MiTSAdTPOG]124 was determined by thermal asymmetric interlaced (TAIL)-PCR (Liu et al., 1995). Two transgenic lines, Tg[MiCiTnIG]2 and Tg[MiCiTnIGCiprmG]2, were used as muscle marker lines (Joly et al., 2007; Sasakura et al., 2008). Three transgenic lines, Tg[MiCiEpiIG]3, Tg[MiCiEpiIG]4 and Tg[MiCiCesACsCesA-CiEpiIG]4, were used as marker lines for the ASP (Joly et al., 2007; Sasakura et al., 2009; Sasakura et al., 2010). The GFP fluorescent images were pseudocolored green.

Plasmids

pRN3CiHox1

The cDNA containing the full open reading frame (ORF) of Ci-Hox1 was amplified by RT-PCR with primers 5′-CCGGATCCCATGAATTCGTACATGAAATACC-3′ and 5′-TTTCACGTGACTATATTCATGTCC-3′. The amplified band was subcloned into the BglII and blunted EcoRI sites of pBS-RN3 (Lemaire et al., 1995) to create pRN3CiHox1.

pSPeCFP-ter

The ORF of eCFP was amplified by PCR with primers 5′-CTGGAATTCTTGTACAGCTCGTCC-3′ and 5′-AGCGGCCGCTATGGTGAGCAAGGGCGA-3′. The PCR fragment was inserted into the NotI and EcoRI sites of pSP-eGFP (Sasakura et al., 2003) to create pSPeCFP-ter.

pSPeCFPCiHox1

An EcoRI fragment of Ci-Hox1 cDNA was inserted into EcoRI site of pSP-eCFP-ter to create pSPeCFPCiHox1. A BamHI fragment of a cis element of Ci-CesA, Ci-AKR and Ci-β2TB were isolated from pCesA(–2080)-GFP (Sasakura et al., 2005), pSPCiAKRK (Hozumi et al., 2010) and pSPCiβ2TBK (Horie et al., 2011), respectively. These cis elements were subcloned into BamHI site of pSPeCFPCiHox1. A cis element of Ci-TTF1 (Satou et al., 2001) was amplified from genomic DNA with primers 5′-TTTTGCGGCCGCCATCTCACAGCAAAGTTTCCAG-3′ and 5′-AAAAGCGGCCGCTAGTTCATGGTTAGCAATGAC-3′, digested with NotI and subcloned into the NotI site of pSPeCFPCiHox1.

Microinjection

The sequence of the antisense morpholino oligonucleotide (MO) for Ci-Hox1 is 5′-AAACTTTACAACTTACTGCTTTTCG-3′. Ci-Hox1 mRNA was synthesized with Megascript T3 kit (Ambion), poly A tailing kit (Ambion) and cap structure analog (New England Biolabs) using pRN3CiHox1 as a template. The concentrations of MO, mRNA and plasmid DNA in the injection medium were 0.5 mM, 200 ng/μl and 1-5 ng/μl, respectively. The sequence of the Raldh antisense MO is 5′-GTACTGCTGATACGACTGAAGACAT-3′. Embryos were treated with U0126 at a concentration of 10 μM.

Quantitative RT-PCR

Total RNA was extracted from juveniles using the AGPC (acid guanidinium-phenol-chloroform) method (Chomczynski and Sacchi, 1987). Genomic DNA was digested with DNaseI (Takara Bio). Reverse transcription was performed with Superscript III reverse transcriptase (Invitrogen) and oligo(dT) primers. Quantitative reverse-transcription (RT)-PCR was carried out with SYBR Premix Ex Taq II (Takara Bio) and a Thermal Cycler Dice Real Time System TP800 (Takara Bio) following the manufacturer’s instructions. EF1α was used as a normalizer gene. The PCR primers for Ci-Hox1 were 5′-AAGCCAACTGTGTTACCACATG-3′ and 5′-ATGTTGTGGCGGATCTTGAAG-3′, and for EF1α they were 5′-CATGTCACGGACAGCGAAACG-3′ and 5′-CAATGTGTGTTGAGGCATTCCAAG-3′.

Whole-mount in situ hybridization

Whole-mount in situ hybridization was carried out as described previously (Yoshida and Sasakura, 2012).

RESULTS AND DISCUSSION

Loss of Ciona Hox1 function results in loss of the gill slit and body wall muscle, and disrupted atrial siphon muscle formation

To investigate the role of the epidermal RA-Hox1 network in chordates, we examined the function of RA-Hox1 in urochordates, the closest evolutionary relatives of vertebrates (Delsuc et al., 2006). Previously, we used transposon-mediated enhancer trapping to create a green fluorescent protein (GFP)-enhancer trap reporter line, EJ[MiTSAdTPOG]124, in the ascidian Ciona intestinalis (Sasakura et al., 2008; Ikuta et al., 2010). In these animals, GFP is expressed in the same pattern as endogenous Ciona intestinalis (Ci-) Hox1 (Fig. 1) (Ikuta et al., 2004) owing to a transposon insertion 192 bp upstream of the Ci-Hox1 transcriptional start site (Fig. 2A). To test whether the insertion disrupts function of the Ci-Hox1 promoter and generates a loss-of-function allele, we generated homozygous animals by crossing two heterozygous EJ[MiTSAdTPOG]124 animals (Fig. 2B-D). The homozygous animals showed notable phenotypes after metamorphosis, including loss of gill slits and body wall muscle (BWM) (Fig. 2B). The mutant was named no gill slit (ngs), after its gill-less phenotype. The ngs mutant phenotype showed the expected Mendelian frequency for a single recessive mutation (supplementary material Table S1), suggesting that a single gene underlies the observed phenotype.

Fig. 1.
Fig. 1.

GFP expression in EJ[MiTSAdTPOG]124 enhancer detection line. (A) Lateral view of a Ciona intestinalis larva (2 days post-fertilization) of EJ[MiTSAdTPOG]124 enhancer detection line. Scale bar: 100 μm. (B) Lateral view of a EJ[MiTSAdTPOG]124 juvenile. GFP is expressed in the posterior part of the endostyle (Es) and digestive tube, including the esophagus (Eso). Scale bar: 100 μm. (C) Ci-Hox1 expression at the juvenile stage. Ci-Hox1 is expressed in the posterior part of the endostyle and posterior part of the intestine including the esophagus. En, endoderm; Ep, epidermis; Nc, nerve cord.

To determine whether Ci-Hox1 is the gene for which function is abrogated in ngs mutants, we examined Ci-Hox1 expression levels in ngs mutant versus control animals by quantitative RT-PCR. ngs mutants showed a dramatic decrease in Ci-Hox1 expression (Fig. 2E). We also knocked down Ci-Hox1 function using an antisense MO that disrupts Ci-Hox1 splicing (supplementary material Fig. S1). Ci-Hox1-MO animals phenocopied ngs mutants (Fig. 2F) and could be rescued by co-injection of Ci-Hox1 mRNA (Fig. 2G). These results indicate that mutation of the Ci-Hox1 gene underlies the ngs phenotype, and that Ci-Hox1 is required for juvenile gill slit and BWM formation.

Fig. 2.
Fig. 2.

Ci-Hox1 is the affected gene in ngs mutants. (A) Insertion site of Minos in the EJ[MiTSAdTPOG]124 transgenic line. Exons are indicated by boxes. Gray and white boxes correspond to the open reading frame and untranslated regions, respectively. (B,C) A wild-type heterozygous Ciona intestinalis juvenile (left) and an ngs mutant (right). Scale bar: 100 μm. (D) Genomic PCR of normal and ngs mutant juveniles. The scheme of the experiment is shown on the left. Bars represent chromosomes and PCR primers are shown by gray arrowheads. Transposon insertions are shown by black arrows. PCR bands were not amplified from the genome of homozygous animals, because long transposon insertion interfered with PCR amplification. Normal juveniles showed PCR bands, whereas ngs mutants showed no PCR band. The lower column is the GAPDH loading control. (E) Quantitative RT-PCR of Ci-Hox1 transcripts. Experiments were performed in duplicate. In ngs mutants, the relative level of Ci-Hox1 mRNA was ∼2-5% that of normal juveniles. (F,G) Juveniles injected with Ci-Hox1 antisense MO (left) or both Ci-Hox1 antisense MO and Ci-Hox1 mRNA (right). Gi, gill slit; BWM, body wall muscle.

To determine whether Ci-Hox1 plays a role in the development of other muscle tissues, we knocked down Ci-Hox1 in transgenic lines expressing GFP in muscles (supplementary material Fig. S2A) (Joly et al., 2007; Sasakura et al., 2008). Formation of the atrial siphon muscle (ASM) was abnormal in these animals, whereas the oral siphon and heart muscles formed normally (supplementary material Fig. S2A,B, Table S2). Although GFP-positive muscle cells were present in the region of the presumptive ASM, they failed to form a ring-shaped, functional ASM muscle. Co-injection of Ci-Hox1 mRNA rescued the Ci-Hox1 MO phenotype (supplementary material Fig. S2C), demonstrating that Ci-Hox1 is required for proper formation of the ASM. Next, we examined whether the BWM and ASM are related to one another as previously suggested (Hirano and Nishida, 1997; Stolfi et al., 2010) by observing formation of the BWM by time-lapse imaging. We found that, indeed, the BWM formed as an extension of the ASM (supplementary material Movie 1). Thus, the absence of the BWM in Ci-Hox1-deficient juveniles is likely to be due to disruption of ASM formation, and a primary function of Ci-Hox1 is ASM formation. Because ASM and heart muscle originate from the same blastomeres (Hirano and Nishida, 1997; Stolfi et al., 2010), Ci-Hox1 should affect ASM formation after the two muscle cells separate.

Ci-Hox1 is necessary for formation of the epidermal structure homologous to the otic placode

In ascidian juveniles, two atrial siphons are formed from the ASP, two thickenings of the larval epidermal ectoderm (Fig. 3A,B). The two atrial siphons then fuse at the midline to form one adult atrial siphon (Berrill, 1947). It has been suggested that the ascidian ASP is homologous to the vertebrate otic placode (Manni et al., 2004; Mazet and Shimeld, 2005; Mazet et al., 2005; Kourakis et al., 2010). In addition, a previous study showed that the ASP is also required for formation of the gill slit (Kourakis and Smith, 2007). To test whether ASP formation is affected in Ci-Hox1-deficient animals, we made use of epidermal GFP transgenic lines (Sasakura et al., 2010) in which the disc-like oral siphon primordium and the ASPs emit stronger GFP fluorescence than do the neighboring epidermal cells (Fig. 3C). In Ci-Hox1 knockdown animals, the ASP was lost, whereas formation of the oral siphon primordium was normal (Fig. 3D; supplementary material Table S3). This phenocopy could be rescued by co-injection of Ci-Hox1 mRNA (Fig. 3E; supplementary material Table S3), indicating that the Ci-Hox1 MO is specific. Taken together, our results demonstrate that Ci-Hox1 is essential for formation first of the ASP and then of the gill slit and ASM/BWM.

Fig. 3.
Fig. 3.

Ci-Hox1 is essential for formation of the ASP. (A) Lateral view of Ciona intestinalis larva with an ASP indicated by a dotted line. (B) Dorsal view of a juvenile. (C) An epidermal GFP transgenic line. (D) A larva injected with Ci-Hox1 antisense MO. No ASP was formed. (E) A larva simultaneously injected with Ci-Hox1 antisense MO and Ci-Hox1 mRNA. Two ASPs were formed. (F) A Ci-Hox1-MO-injected larva in which Ci-Hox1 is overexpressed in the epidermis. ASPs were formed. (G) A Ci-Hox1-MO-injected larva in which Ci-Hox1 was overexpressed in the CNS. ASPs were not formed. (H) A Ci-Hox1-MO-injected larva in which Ci-Hox1 was overexpressed in the mesenchyme. ASPs were not formed. (I) A Ci-Hox1-MO-injected larva in which Ci-Hox1 was overexpressed in the endoderm. ASPs were not formed. (J) A Raldh-MO-injected larva. ASPs were not formed. (K) A Raldh-MO-injected larva in which Ci-Hox1 was overexpressed in the epidermis. Two ASPs were formed. as, atrial siphon; osp, oral siphon primordium. Scale bars: 100 μm.

Ci-Hox1 is expressed in several tissues at the larval stage, including the epidermal ectoderm, CNS and endoderm (Ikuta et al., 2004). To determine which expression domain of Ci-Hox1 is responsible for ASP formation, we generated tissue-specific Ci-Hox1 expression constructs and tested their ability to rescue the Ci-Hox1-MO ASP phenocopy. Strong rescue was observed when Ci-Hox1 was expressed in the epidermal ectoderm (Fig. 3F; supplementary material Table S3). This result indicates that expression of Ci-Hox1 in the epidermal ectoderm is required for formation of the ASP. As two properly positioned ASPs were formed even though Ci-Hox1 was overexpressed throughout the embryo body, which was shown by rescue experiment of Ci-Hox1 MO phenocopy with Ci-Hox1 mRNA, RA-driven Ci-Hox1 might render the epidermis competent to respond to the ASP-inducing signals. In contrast to the epidermis, expression of Ci-Hox1 in the CNS and mesenchyme failed to rescue the MO phenocopy (Fig. 3G,H; supplementary material Table S3). A moderate rescue was observed when Ci-Hox1 was expressed in the endoderm (Fig. 3I; supplementary material Table S3), suggesting that Ci-Hox1 in the endoderm has a role in formation of the ASP.

Kourakis and Smith (Kourakis and Smith, 2007) previously suggested that FGF/MEK signaling after the early tailbud stage serves to induce the ASP. If Ci-Hox1 gives the epidermal ectoderm competence to respond to the inductive signal of the ASP, expression of Ci-Hox1 in the epidermis should be independent of the inductive signal. Ci-Hox1 expression is observed in the epidermis at the early tailbud stage, which is earlier than the induction of the ASP, suggesting that Ci-Hox1 expression is independent of the inductive signal. To address the independence between Ci-Hox1 in the epidermis and inductive signaling of ASP, we treated embryos with U0126 from the early tailbud stage, causing loss of the ASP (supplementary material Table S4). Microinjection of Ci-Hox1 mRNA failed to overcome the effect (supplementary material Table S4), suggesting that inductive signaling of the ASP is not mediated by Ci-Hox1 in the epidermal ectoderm.

Retinoic acid-driven epidermal expression of Hox1 is necessary for ASP formation

The expression of Ci-Hox1 in the epidermal ectoderm is directly upregulated by RA (Ishibashi et al., 2005; Kanda et al., 2009). To test the possibility that RA is involved in ASP formation, we disrupted RA synthesis by knocking down the gene encoding retinal dehydrogenase (Raldh), an RA synthesis enzyme (Niederreither et al., 1999), with an antisense MO. Raldh-MO larvae exhibited loss of the ASP (Fig. 3J; supplementary material Table S5), suggesting that RA is necessary for ASP formation. When Ci-Hox1 was overexpressed in the epidermis of Raldh-MO larvae, the phenotype was rescued and ASP formation was observed (Fig. 3K; supplementary material Table S5). These results indicate that RA functions in ASP formation via epidermal expression of Ci-Hox1.

Conclusions

We conclude that RA-driven Hox1 expression in the epidermal ectoderm is essential for organizing the ASP/otic placode in the urochordate Ciona intestinalis (Fig. 4). In addition, this network functions directly in the ASP/otic placode to pattern it. Similarly, in amphioxus, RA functions in patterning of the epidermal sensory organ (Schubert et al., 2004), from which placodes are thought to originate (Holland and Holland, 2001). In vertebrates, otic placode formation depends on signals from a properly patterned CNS (Hans and Westerfield, 2007), and is therefore indirectly dependent on RA and Hox1. However, expression of Hoxa1 in the otic epithelium (Makki and Capecchi, 2010) raises the possibility that the RA-Hox1 network might also function in the epidermal ectoderm to form the otic placode in vertebrates. Furthermore, Hox1 expression in the epidermal ectoderm is observed in hemichordates (Aronowicz and Lowe, 2006). Thus, the role of RA-Hox1 in specification of the epidermal sensory organ might have been inherited from the deuterostome ancestor of chordates and recruited for otic placode formation in the urochordate/vertebrate lineages. Because both the dorsal position of the CNS and the epidermally specialized placodes are hallmarks of chordates, the RA-Hox1 network appears to have played key roles in these evolutionary innovations crucial for acquiring the chordate body plan. Our study also suggests that Ci-Hox1 in the endoderm functions in ASP formation. In Ciona, the inductive signal for ASP formation is thought to be mediated by fibroblast growth factor (FGF) signaling (Kourakis and Smith, 2007). Although the source of the FGF signal has not been uncovered, the endoderm is a good candidate. Because Ci-Hox1 is probably the competence factor for ASP/otic placode formation, Ci-Hox1 might be upstream of the transcription factor genes expressed preferably in the placode, such as FoxIa, Pax2/5/8, eyes absent and Six1/2 (Mazet and Shimeld, 2005). This issue also needs to be investigated for understanding the mechanisms underlying formation of the ASP/otic placode.

Fig. 4.
Fig. 4.

A model summarizing the relationship between Ci-Hox1 and the inductive signal of the ASP. RA drives Ci-Hox1 expression (purple) in the epidermis. The epidermis acquires competence to receive the inductive signal, and two ASPs are formed. In Ci-Hox1-mutant or morphant embryos, the epidermis cannot receive the inductive signal, and no ASP was formed.

Acknowledgments

We thank the National Bioresource Project, MEXT, and all members of the Maizuru Fishery Research Station of Kyoto University and the Education and Research Center of Marine Bioresources of Tohoku University for providing us with Ciona adults.

Footnotes

  • Funding

    This study was supported by Grants-in-Aid for Scientific Research from the Japan Society for the Promotion of Science (JSPS) and the Ministry of Education, Culture, Sports, Science and Technology (MEXT) to Y.S., T.H., N.S. and S.F. Y.S. was supported by the National Institute of Genetics Cooperative Research Program [2009-B01].

  • Competing interests statement

    The authors declare no competing financial interests.

  • Supplementary material

    Supplementary material available online at http://dev.biologists.org/lookup/suppl/doi:10.1242/dev.080234/-/DC1

  • Accepted April 8, 2012.

References

  1. ↵
    1. Aronowicz J.,
    2. Lowe C.
    (2006). Hox gene expression in the hemichordate Saccoglossus kowalevskii and the evolution of deuterostome nervous system. Int. Comp. Biol. 46, 890–901.
    OpenUrlAbstract/FREE Full Text
  2. ↵
    1. Awazu S.,
    2. Matsuoka T.,
    3. Inaba K.,
    4. Satoh N.,
    5. Sasakura Y.
    (2007). High-throughput enhancer trap by remobilization of transposon Minos in Ciona intestinalis. Genesis 45, 307–317.
    OpenUrlCrossRefPubMed
  3. ↵
    1. Berrill N. J.
    (1947). Development of Ciona. J. Mar. Biol. Assoc. 26, 616–625.
    OpenUrlCrossRef
  4. ↵
    1. Chomczynski P.,
    2. Sacchi N.
    (1987). Single-step method of RNA isolation by acid guanidium thiocyanate-phenol-chloroform extraction. Anal. Biochem. 162, 156–159.
    OpenUrlCrossRefPubMedWeb of Science
  5. ↵
    1. Delsuc F.,
    2. Brinkmann H.,
    3. Chourrout D.,
    4. Philippe H.
    (2006). Tunicates and not cephalochordates are the closest living relatives of vertebrates. Nature 439, 965–968.
    OpenUrlCrossRefPubMedWeb of Science
  6. ↵
    1. Gavalas A.,
    2. Krumlauf R.
    (2000). Retinoid signalling and hindbrain patterning. Curr. Opin. Genet. Dev. 10, 380–386.
    OpenUrlCrossRefPubMedWeb of Science
  7. ↵
    1. Hans S.,
    2. Westerfield M.
    (2007). Changes in retinoic acid signaling alter otic patterning. Development 134, 2449–2458.
    OpenUrlAbstract/FREE Full Text
  8. ↵
    1. Hirano T.,
    2. Nishida H.
    (1997). Developmental fates of larval tissues after metamorphosis in ascidian Halocynthia roretzi. I. Origin of mesodermal tissues of the juvenile. Dev. Biol. 192, 199–210.
    OpenUrlCrossRefPubMedWeb of Science
  9. ↵
    1. Holland L. Z.
    (2005). Non-neural ectoderm is really neural: evolution of developmental patterning mechanisms in the non-neural ectoderm of chordates and the problem of sensory cell homologies. J. Exp. Zool. B Mol. Dev. Evol. 304, 304–323.
    OpenUrlPubMed
  10. ↵
    1. Holland L. Z.,
    2. Holland N. D.
    (2001). Evolution of neural crest and placodes: amphioxus as a model for the ancestral vertebrate? J. Anat. 199, 85–98.
    OpenUrlPubMedWeb of Science
  11. ↵
    1. Horie T.,
    2. Shinki R.,
    3. Ogura Y.,
    4. Kusakabe T.,
    5. Satoh N.,
    6. Sasakura Y.
    (2011). Ependymal cells of chordate larvae are stem-like cells that form the adult nervous system. Nature 469, 525–528.
    OpenUrlCrossRefPubMed
  12. ↵
    1. Hozumi A.,
    2. Kawai N.,
    3. Yoshida R.,
    4. Ogura Y.,
    5. Ohta N.,
    6. Satake H.,
    7. Satoh N.,
    8. Sasakura Y.
    (2010). Efficient transposition of a single Minos transposon copy in the genome of the ascidian Ciona intestinalis with a transgenic line expressing transposase in eggs. Dev. Dyn. 239, 1076–1088.
    OpenUrlCrossRefPubMed
  13. ↵
    1. Ikuta T.,
    2. Yoshida N.,
    3. Satoh N.,
    4. Saiga H.
    (2004). Ciona intestinalis Hox gene cluster: Its dispersed structure and residual colinear expression in development. Proc. Natl. Acad. Sci. USA 101, 15118–15123.
    OpenUrlAbstract/FREE Full Text
  14. ↵
    1. Ikuta T.,
    2. Satoh N.,
    3. Saiga H.
    (2010). Limited functions of Hox genes in the larval development of the ascidian Ciona intestinalis. Development 137, 1505–1513.
    OpenUrlAbstract/FREE Full Text
  15. ↵
    1. Ishibashi T.,
    2. Usami T.,
    3. Fujie M.,
    4. Azumi K.,
    5. Satoh N.,
    6. Fujiwara S.
    (2005). Oligonucleotide-based microarray analysis of retinoic acid target genes in the protochordate, Ciona intestinalis. Dev. Dyn. 233, 1571–1578.
    OpenUrlCrossRefPubMed
  16. ↵
    1. Joly J. S.,
    2. Kano S.,
    3. Matsuoka T.,
    4. Auger H.,
    5. Hirayama K.,
    6. Satoh N.,
    7. Awazu S.,
    8. Legendre L.,
    9. Sasakura Y.
    (2007). Culture of Ciona intestinalis in closed systems. Dev. Dyn. 236, 1832–1840.
    OpenUrlCrossRefPubMedWeb of Science
  17. ↵
    1. Kanda M.,
    2. Wada H.,
    3. Fujiwara S.
    (2009). Epidermal expression of Hox1 is directly activated by retinoic acid in the Ciona intestinalis embryo. Dev. Biol. 335, 454–463.
    OpenUrlCrossRefPubMed
  18. ↵
    1. Kourakis M. J.,
    2. Smith W. C.
    (2007). A conserved role for FGF signaling in chordate otic/atrial placode formation. Dev. Biol. 312, 245–257.
    OpenUrlCrossRefPubMed
  19. ↵
    1. Kourakis M. J.,
    2. Newman-Smith E.,
    3. Smith W. C.
    (2010). Key steps in the morphogenesis of a cranial placode in an invertebrate chordate, the tunicate Ciona savignyi. Dev. Biol. 340, 134–144.
    OpenUrlCrossRefPubMed
  20. ↵
    1. Lemaire P.,
    2. Garrett N.,
    3. Gurdon J. B.
    (1995). Expression cloning of Siamois, a Xenopus homeobox gene expressed in dorsal-vegetal cells of blastulae and able to induce a complete secondary axis. Cell 81, 85–94.
    OpenUrlCrossRefPubMedWeb of Science
  21. ↵
    1. Liu Y. G.,
    2. Mitsukawa N.,
    3. Oosumi T.,
    4. Whittier R. F.
    (1995). Efficient isolation and mapping of Arabidopsis thaliana T-DNA insert junctions by thermal asymmetric interlaced PCR. Plant J. 8, 457–463.
    OpenUrlCrossRefPubMedWeb of Science
  22. ↵
    1. Makki N.,
    2. Capecchi M. R.
    (2010). Hoxa1 lineage tracing indicates a direct role for Hoxa1 in the development of the inner ear, the heart, and the third rhombomere. Dev. Biol. 341, 499–509.
    OpenUrlCrossRefPubMed
  23. ↵
    1. Manni L.,
    2. Lane N.,
    3. Joly J.,
    4. Gasparini F.,
    5. Tiozzo S.,
    6. Caicci F.,
    7. Zaniolo G.,
    8. Burighel P.
    (2004). Neurogenic and non-neurogenic placodes in ascidians. J. Exp. Zool. B Mol. Dev. Evol. 302, 483–504.
    OpenUrl
  24. ↵
    1. Mark M.,
    2. Lufkin T.,
    3. Vonesch J. L.,
    4. Ruberte E.,
    5. Olivo J. C.,
    6. Dolle P.,
    7. Gorry P.,
    8. Lumsden A.,
    9. Chambon P.
    (1993). Two rhombomeres are altered in Hoxa-1 mutant mice. Development 119, 319–338.
    OpenUrlAbstract
  25. ↵
    1. Mazet F.,
    2. Shimeld S. M.
    (2005). Molecular evidence from ascidians for the evolutionary origin of vertebrate cranial sensory placodes. J. Exp. Zool. B Mol. Dev. Evol. 304, 340–346.
    OpenUrlPubMed
  26. ↵
    1. Mazet F.,
    2. Hutt J. A.,
    3. Milloz J.,
    4. Millard J.,
    5. Graham A.,
    6. Shimeld S. M.
    (2005). Molecular evidence from Ciona intestinalis for the evolutionary origin of vertebrate sensory placodes. Dev. Biol. 282, 494–508.
    OpenUrlCrossRefPubMedWeb of Science
  27. ↵
    1. McGinnis W.,
    2. Krumlauf R.
    (1992). Homeobox genes and axial patterning. Cell 68, 283–302.
    OpenUrlCrossRefPubMedWeb of Science
  28. ↵
    1. Niederreither K.,
    2. Subbarayan V.,
    3. Dolle P.,
    4. Chambon P.
    (1999). Embryonic retinoic acid synthesis is essential for early mouse post-implantation development. Nat. Genet. 21, 444–448.
    OpenUrlCrossRefPubMedWeb of Science
  29. ↵
    1. Sasakura Y.,
    2. Awazu S.,
    3. Chiba S.,
    4. Satoh N.
    (2003). Germ-line transgenesis of the Tc1/mariner superfamily transposon Minos in Ciona intestinalis. Proc. Natl. Acad. Sci. USA 100, 7726–7730.
    OpenUrlAbstract/FREE Full Text
  30. ↵
    1. Sasakura Y.,
    2. Nakashima K.,
    3. Awazu S.,
    4. Matsuoka T.,
    5. Nakayama A.,
    6. Azuma J.,
    7. Satoh N.
    (2005). Transposon-mediated insertional mutagenesis revealed the functions of animal cellulose synthase in the ascidian Ciona intestinalis. Proc. Natl. Acad. Sci. USA 102, 15134–15139.
    OpenUrlAbstract/FREE Full Text
  31. ↵
    1. Sasakura Y.,
    2. Konno A.,
    3. Mizuno K.,
    4. Satoh N.,
    5. Inaba K.
    (2008). Enhancer detection in the ascidian Ciona intestinalis with transposase-expressing lines of Minos. Dev. Dyn. 237, 39–50.
    OpenUrlCrossRefPubMed
  32. ↵
    1. Sasakura Y.,
    2. Inaba K.,
    3. Satoh N.,
    4. Kondo M.,
    5. Akasaka K.
    (2009). Ciona intestinalis and Oxycomanthus japonicus, representatives of marine invertebrates. Exp. Anim. 58, 459–469.
    OpenUrlCrossRefPubMed
  33. ↵
    1. Sasakura Y.,
    2. Suzuki M. M.,
    3. Hozumi A.,
    4. Inaba K.,
    5. Satoh N.
    (2010). Maternal factor-mediated epigenetic gene silencing in the ascidian Ciona intestinalis. Mol. Genet. Genomics 283, 99–110.
    OpenUrlCrossRefPubMed
  34. ↵
    1. Satou Y.,
    2. Imai K. S.,
    3. Satoh N.
    (2001). Early embryonic expression of a LIM-homeobox gene Cs-lhx3 is downstream of β-catenin and responsible for the endoderm differentiation in Ciona savignyi embryos. Development 128, 3559–3570.
    OpenUrlAbstract/FREE Full Text
  35. ↵
    1. Schubert M.,
    2. Holland N. D.,
    3. Escriva H.,
    4. Holland L. Z.,
    5. Laudet V.
    (2004). Retinoic acid influences anteroposterior positioning of epidermal sensory neurons and their gene expression in a developing chordate (amphioxus). Proc. Natl. Acad. Sci. USA 101, 10320–10325.
    OpenUrlAbstract/FREE Full Text
  36. ↵
    1. Shimeld S. M.,
    2. Holland P. W.
    (2000). Vertebrate innovations. Proc. Natl. Acad. Sci. USA 97, 4449–4452.
    OpenUrlAbstract/FREE Full Text
  37. ↵
    1. Stolfi A.,
    2. Gainous B.,
    3. Young J. J.,
    4. Mori A.,
    5. Levine M.,
    6. Christiaen L.
    (2010). Early chordate origins of the vertebrate second heart field. Science 329, 565–568.
    OpenUrlAbstract/FREE Full Text
  38. ↵
    1. Yoshida R.,
    2. Sasakura Y.
    (2012). Establishment of the enhancer detection lines expressing GFP in the gut of the ascidian Ciona intestinalis. Zool. Sci. 29, 11–20.
    OpenUrlCrossRefPubMed
Back to top

 Download PDF

Email
Research Report
Retinoic acid-driven Hox1 is required in the epidermis for forming the otic/atrial placodes during ascidian metamorphosis
Yasunori Sasakura, Miyuki Kanda, Taku Ikeda, Takeo Horie, Narudo Kawai, Yosuke Ogura, Reiko Yoshida, Akiko Hozumi, Nori Satoh, Shigeki Fujiwara
Development 2012 139: 2156-2160; doi: 10.1242/dev.080234
del.icio.us logo Digg logo Reddit logo Twitter logo CiteULike logo Facebook logo Google logo Mendeley logo
Citation Tools
Alerts

Article navigation

Other journals from The Company of Biologists

Advertisement

An interview with Swathi Arur

Swathi Arur joined the team at Development as an Academic Editor in 2020. Her lab uses multidisciplinary approaches to understand female germline development and fertility. We met with her over Zoom to hear more about her life, her career and her love for C. elegans.

Jim Wells and Hanna Mikkola join our team of Editors

We are pleased to welcome James (Jim) Wells and Hanna Mikkola to our team of Editors. Jim joins us a new Academic Editor, taking over from Gordan Keller, and Hanna joins our team of Associate Editors. Find out more about their research interests and areas of expertise.

New funding scheme supports sustainable events

As part of our Sustainable Conferencing Initiative, we are pleased to announce funding for organisers that seek to reduce the environmental footprint of their event. The next deadline to apply for a Scientific Meeting grant is 26 March 2021.

Read & Publish participation continues to grow

“I’d heard of Read & Publish deals and knew that many universities, including mine, had signed up to them but I had not previously understood the benefits that these deals bring to authors who work at those universities.”

Professor Sally Lowell (University of Edinburgh) shares her experience of publishing Open Access as part of our growing Read & Publish initiative. We now have over 150 institutions in 15 countries and four library consortia taking part – find out more and view our full list of participating institutions.

Upcoming special issues

Imaging Development, Stem Cells and Regeneration
Submission deadline: 30 March 2021
Publication: mid-2021

The Immune System in Development and Regeneration
Guest editors: Florent Ginhoux and Paul Martin
Submission deadline: 1 September 2021
Publication: Spring 2022

Both special issues welcome Review articles as well as Research articles, and will be widely promoted online and at key global conferences.

Development presents...

Our successful webinar series continues into 2021, with early-career researchers presenting their papers and a chance to virtually network with the developmental biology community afterwards. Here, Brandon Carpenter talks about how inherited histone methylation defines the germline versus soma decision in C. elegans. 

Sign up to join our next session:

10 March
Time: TBC
Chaired by: Thomas Lecuit