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Novel developmental bases for the evolution of hypobranchial muscles in vertebrates

Abstract

Background

Vertebrates are characterized by possession of hypobranchial muscles (HBMs). Cyclostomes, or modern jawless vertebrates, possess a rudimentary and superficial HBM lateral to the pharynx, whereas the HBM in jawed vertebrates is internalized and anteroposteriorly specified. Precursor cells of the HBM, marked by expression of Lbx1, originate from somites and undergo extensive migration before becoming innervated by the hypoglossal nerve. How the complex form of HBM arose in evolution is relevant to the establishment of the vertebrate body plan, but despite having long been assumed to be similar to that of limb muscles, modification of developmental mechanisms of HBM remains enigmatic.

Results

Here we characterize the expression of Lbx genes in lamprey and hagfish (cyclostomes) and catshark (gnathostome; jawed vertebrates). We show that the expression patterns of the single cyclostome Lbx homologue, Lbx-A, do not resemble the somitic expression of mammalian Lbx1. Disruption of Lbx-A revealed that LjLbx-A is required for the formation of both HBM and body wall muscles, likely due to the insufficient extension of precursor cells rather than to hindered muscle differentiation. Both homologues of Lbx in the catshark were expressed in the somitic muscle primordia, unlike in amniotes. During catshark embryogenesis, Lbx2 is expressed in the caudal HBM as well as in the abdominal rectus muscle, similar to lamprey Lbx-A, whereas Lbx1 marks the rostral HBM and pectoral fin muscle.

Conclusions

We conclude that the vertebrate HBM primarily emerged as a specialized somatic muscle to cover the pharynx, and the anterior internalized HBM of the gnathostomes is likely a novelty added rostral to the cyclostome-like HBM, for which duplication and functionalization of Lbx genes would have been a prerequisite.

Background

Many characteristics of vertebrate body plan are associated with the extremely complex morphology of skeletal muscles, as compared to the simple contractile tissues of invertebrate chordates, such as those found in amphioxus. Of the vertebrate skeletal muscles, hypobranchial muscles (HBMs), including tongue and infrahyoid muscles in jawed vertebrates, have attracted particular attention in evolutionary studies, due to their peculiar developmental processes. Precursor cells of the HBM originate from somites and migrate along an extensive, arch-shaped pathway circumventing the posterior margin of the posteriormost pharyngeal arch, as a cell stream called the hypoglossal cord [1]. HBMs become innervated by the hypoglossal nerve, the twelfth cranial nerve that runs through the so-called head/trunk interface, overlapping with the hypoglossal cord [2].

The extensive migration of the somitic muscle precursors has been best studied in the formation of paired limbs, another feature shared by vertebrates. At the fore- and hindlimb levels, the ventrolateral lip (VLL) of the epithelial dermomyotome yields de-epithelialized, mesenchymal precursor cells for the limb muscles. The limb muscle precursors lose their original segmental configuration, forming a pool of mesenchymal progenitor cells that migrate distally into the limb buds, where they undergo muscle differentiation [3]. These precursor cells are marked by the expression of Lbx1, a member of lady bird class of homeobox transcription factor-encoding genes [4, 5]. In Lbx1-deficient mice, the limb muscles are lost or severely affected, with tongue muscles reduced in size [5, 6]. However, Lbx2, a paralogue of Lbx1, has never been proposed to be involved in myogenesis in either tongue or limbs [7,8,9].

In recent developmental studies, the cyclostome lampreys have served as an attractive model that retains the ancestral features of vertebrates [10,11,12,13,14]. One such characteristic is found in the simple morphology of skeletal muscles, e.g., a lack of epaxial/hypaxial distinction of the trunk muscles, as well as the paired fins and associated muscles [15, 16]. On the other hand, lampreys, while lacking the tongue, do possess a putative HBM homologue lying in the superficial layer of the pharyngeal wall, innervated by a nerve called the hypoglossal nerve (XII) in the lamprey (Fig. 1a) [18, 19]. Precursors of the lamprey HBM appear to originate from the ventral side of rostral somites of the late pharyngula (stage 27) [20], first migrating ventrally within the pericardium and then extending anteriorly along the lateral aspect of the pharynx [11, 18, 21,22,23]. Muscle differentiation of HBMs takes place at the pre-ammocoete larval stage (stage 29; Additional file 1: Fig. S1j), much later than that of other somite-derived muscles. Upon differentiation, HBM myofibers secondarily acquire segmental pattern in conjunction with the pharyngeal arch muscles that derive from unsegmented head mesoderm (Additional file 1: Fig. S1b-f), but not in conjunction with segmentation of the dorsal somitic muscles dorsally overlying the pharyngeal arches (Additional file 1: Fig. S1k and l) [10, 22].

Fig. 1
figure1

Lbx-A gene in expression in lamprey and hagfish embryos. a A pre-ammocoete larva doubly stained with phalloidin (green; skeletal muscles) and acetylated tubulin antibody (green; neurons). HBM, hypobranchial muscle; m, mouth; XII, hypoglossal nerve. be Expression of LjLbx-A gene in the rostral part of lamprey embryos. Arrowheads indicate the rostral end of hypobranchial muscle (HBM) primordia. Arrows indicate the ventral edge of the extending body wall muscle primordia. b, d Left lateral views. c Ventral view. e Left-ventral view. f Differentiated somitic muscles visualized by myosin heavy chain antibody MF20. gl Anterior portion of the stage 30 embryos stained with MyHC antibody MF20, viewed from the left (g, i, k) and right (h, j, l) sides. Compared to the embryos injected with Cas9 only (g, h), LjLbx-A-disrupted embryos have thinner and shorter HBM (il). m 3D reconstruction of an HE-stained stage 53 hagfish embryo showing location of the hypobranchial-equivalent muscle anlage (dark green; Oisi et al. [17]). Dorsolateral segmented muscles (m. par) are shown by the repeated pattern of light greens. m. obl/rect, anterior oblique muscles and the rectus muscles; m. par, parietal muscles. n, o Expression of EbLbx-A in the trunk of stage 53 hagfish embryo. Arrowheads show the expression at the ventral edge of the somites. Transverse sections at pharyngeal (n) and cloacal (o) levels. no, notochord; nt, neural tube. Scale bars, 200 mm

The lampreys, as well as the hagfish, the other group making up the cyclostomes, possess a single cyclostome-specific homologue of the Lbx gene, Lbx-A (Fig. S2). In the Japanese lamprey Lethenteron camtschaticum (formerly Lethenteron japonicum), Lbx-A (LjLbx-A) mRNA has been shown to mark the anteriorly extending HBM precursors [10]. This observation led us to speculate that LjLbx-A would retain the ancestral myogenic function of Lbx gene in HBM formation acquired early in vertebrate evolution. However, it remains unclear how Lbx1/Lbx2 genes of gnathostomes are functionally related to the single Lbx gene of the lamprey. In this study, we aimed to clarify how the duplicated Lbx genes are involved in the morphological complexity of gnathostome HBM by comparing myogenesis in the lamprey, hagfish, and shark.

Results and discussion

Characterization and functional analysis of the cyclostome Lbx-A genes

In the present study, we first examined the functional importance of lamprey Lbx-A gene during development. Since LjLbx-A sequence reported previously had lacked the 5′ part of the coding region [10], we isolated a full-length cDNA clone of LjLbx-A utilizing the updated genomic data and the gene modeling (Additional file 1: Fig. S2). Newly identified N-terminus of deduced amino acid sequence of LjLbx-A contained a 6-amino acid lady bird domain which is shared with Drosophila lady bird and mammalian Lbx2 genes, but not with mammalian Lbx1 genes, implicating a possible functional correlation of LjLbx-A to Lbx2 genes of jawed vertebrates [24].

We subsequently carried out the detailed analyses of the expression of LjLbx-A. In addition to the expression in HBM (Fig. 1b–d), LjLbx-A was also expressed in the ventral edge of the postotic trunk somites across the anteroposterior axis, in addition to the HBM precursor cells (Fig. 1e). These LjLbx-A-expressing cells in the trunk extend ventrally to form the body wall muscle (stage 29; Additional file 1: Fig. S1j), differentiating much later than the dorsal part of the trunk muscle (Fig. 1f, Additional file 1: Fig. S1g-j). In the later ammcoete larval stage (~ 50 mm body length), LjLbx-A was expressed in a cell layer at the dorsal edge of the myotomes, which would later give rise to the muscles in the dorsal median fin (Additional file 1: Fig. S4) [25].

The broad expression of LjLbx-A in the ventral side of the trunk does not resemble the somitic expression of mammalian Lbx1, which is expressed only in the occipital and limb levels, but not in the flank [4, 26]. To clarify which of the lamprey larval muscles require the function of LjLbx-A, we disrupted the LjLbx-A locus during embryogenesis, using CRISPR/Cas9-mediated gene editing (Fig. 1g-l, Additional file 1: Fig. S5 to S8). After injection of the Cas9 protein and gRNA complementary to LjLbx-A, the dorsal somitic muscles of the larvae appeared unaffected, whereas HBM was lost partly or entirely from the ventral floor of the pharynx (Fig. 1g-l, Additional file 1: Fig. S6a-c). These embryos also lost body wall muscles, suggesting that LjLbx-A is required for the formation of both HBM and body wall muscles (Additional file 1: Fig. S6d-f). We also found that LjLbx-A-depleted embryos lost the expression of LjPax3/7-A in the pharyngeal region, which marks the extending HBM primordium (Additional file 1: Fig. S7) [10, 23], suggesting that the loss of HBM and body wall muscles is attributable to the insufficient extension of precursor cells rather than to hindered muscle differentiation.

We also characterized the Lbx gene of the hagfish Eptatretus burgeri, EbLbx-A (Additional file 1: Fig. S3). In hagfish embryos, EbLbx-A was expressed in the ventral edge of the somites (Fig. 1n, o) [17]. This region has been reported to give rise to the anterior oblique muscles (m. decussatus) and the rectus muscles in the ventrolateral aspect of the pharyngeal wall (m. obl/rect; Fig. 1m) [17]. M. obl/rect have been proposed to characterize the HBM of the hagfish, despite the fact that these muscles are innervated by the occipitospinal nerves that pass ventrally as individual segmental nerves, not by a bundled hypoglossal nerve which is the case in the lamprey HBM (Fig. 1a). The morphology of hagfish m. obl/rect also differs significantly from that of the lamprey HBM; the oblique muscles broadly cover the surface of the ventral body from caudal to the mouth to the cloaca, and the rectus muscles lie longitudinally close to the ventral midline. Nevertheless, m. obl/rect have been reported to differentiate at a later stage of embryogenesis [17], which is also the case in the development of the lamprey HBM and body wall muscles (Additional file 1: Fig. S1). The fact that the expression of EbLbx-A is restricted to the ventral somites supports the HBM nature of the m. obl/rect, suggesting that the Lbx-dependent regulation of differentiation would be conserved in the cyclostomes.

Catshark Lbx1 and Lbx2 are differentially expressed during myogenesis

We chose the elasmobranch cloudy catshark Scyliorhinus torazame as a model to investigate how the wide variety of somite-derived hypaxial muscles, such as those in the limbs, appeared in the vertebrate species diverged early in evolution. It has been reported that, similarly to those of Osteichthyan animals, the Lbx1 gene of shark and skates are expressed in precursor cells in muscles [27, 28]. However, involvement of Lbx2 in myogenesis in these animals had remained unexplored, and no insights had been obtained with respect to the differential expression of Lbx1 and Lbx2, which emerged possibly due to the two rounds of vertebrate whole genome duplication (Additional file 1: Fig. S3) [27, 29]. In this study, we examined the expression of Lbx1 and Lbx2 during embryogenesis of S. torazame, using probes specific to each of the two genes. Unlike in mammals, both Lbx1 and Lbx2 were expressed in the somitic muscle primordia, although in a non-overlapping fashion, as detailed below (Fig. 2).

Fig. 2
figure2

Expression of Lbx1 and Lbx2 in S. torazame. Expression of Lbx1 (ad) and Lbx2 (eg) detected by whole-mount in situ hybridization. Arrowhead and arrows indicate the patch of Lbx1 expression in CMD and paired fin muscle primordia, respectively. Scale bars, 0.5 mm (a, b, e, f), 1 mm (c, g), and 2 mm (d)

Expression of catshark Lbx1 commenced at the epithelial VLL of postotic somites and became restricted to the pectoral and pelvic fin levels (Fig. 2a–c). Near the fin buds, these Lbx1-positive cells detached from the VLL in bulk, in a similar configuration to the “muscle bud” described by Goodrich (Fig. 3a) [30, 31], to invade the fin bud, where they differentiated into adductor and abductor muscles of the paired fins (Figs. 2a–d and 3d, g, j). Remarkably, these cell aggregates maintained their initial somitomeric pattern and were positive for ZO-1 (zona occuludens-1) antibody, a marker for tight junctions, suggesting that the dermomyotome persisting in the fin muscle primordia is epithelial in nature (Fig. 3e) [32, 33]. This observation is consistent with the classical view that the chondrichthyan fin muscles form from epithelial muscle primordium [30]. Lbx1 was also expressed in the muscle primordia in median fins (Figs. 2d and 3k, l), similarly to the case in LjLbx-A (Additional file 1: Fig. S4).

Fig. 3
figure3

Shark Lbx1 and Lbx2 are expressed in distinct muscle primordium in the trunk. Transverse sections of S. torazame embryos at ac stage 27, df stage 28, and gi stage 29. a Expression of Lbx1 detected in the pectoral muscle precursor cells (arrows). b A serial section to a, Lbx2 is expressed in the ventral somite in the body wall. c At the pectoral fin level, Lbx2 is expressed in rectus abdominus muscle primordia (dotted bracket), which is not yet differentiated, as shown by the absence of MyHC staining (c). d, e Lbx1 is expressed in the pectoral fin muscle primordia (arrow) which is also stained with ZO-1 tight junction antibody. gi At stage 29, Lbx1 is expressed in the pectral fin muscle primordia which are still not differentiated. Expression of Lbx2 is no longer detectable. Muscle differentiation is observed only in the rectus abdominus (dotted bracket) but not yet in the fin (i). j, k At stage 32, muscle differentiation is observed in the appendicular (arrow in j) and median (arrow in k) fins. l At stage 29, Lbx1 is expressed in the muscle precursor cells in the dorsal median fin (arrow). Scale bars, a, d, g 0.1 mm; j, k 0.5 mm; l 0.05 mm

Catshark Lbx1 was not expressed in the abdominal muscle primordia (Fig. 3a, g), unlike lamprey/hagfish Lbx-A. Remarkably, in contrast to the Lbx1, catshark Lbx2 continued to be expressed in the VLL throughout the trunk (Figs. 2e–g and 3b). Lbx2-positive cells did not enter the fin buds; Lbx2-positive VLL cells extended ventromedially, passing through the medial aspect of the fin buds (Fig. 3b, f), marking the future abdominal rectus muscle (Fig. 3i). Thus, catshark Lbx2, but not Lbx1, marks the developing abdominal muscle, a feature similar to that of lamprey Lbx-A described above (Fig. 1e).

Catshark HBM exhibits differential expression of Lbx1 and Lbx2 during HBM development

Our observations also suggested the differential functions of Lbx1 and Lbx2 in HBM development in S. torazame (Fig. 4). In early embryos, Lbx2 is expressed in a projection of the cells originating from the anterior somites (Fig. 4a, b, Additional file 1: Fig. S9a). The epithelial VLL of the 3rd and 4th somites released the Lbx2-positive cells ventrally along the posterior edge of the pharynx (Additional file 1: Fig. S9a-c). Later, the Lbx2-positive cells accumulated adjacent to the heart, then further proceeded anteriorly within the body wall ventral to the pharynx (Fig. 4a, b; Additional file 1: Fig. S9d-f). In contrast, the expression of Lbx1 was not consecutive along the posterior circumference of the pharynx. At stage 28, a single patch of Lbx1 expression became evident at the level of the 3rd pharyngeal arch (arrowhead in Figs. 2c and 4c, d, e’). This expression of Lbx1 in the anteriormost part of HBM primordium did not overlap with the Lbx2 expression in the midline, whereas dorsally the leading edges of the bilateral portion of HBM transiently express both Lbx1 and Lbx2 (Fig. 4f’ and f”). During the extension of HBM primordium from the somites, the anteriormost portion of Lbx2-positive domain seems to provide Lbx1-positive precursor cells to give rise to the anterior HBM that fuses in the midline.

Fig. 4
figure4

Anterior part of the shark hypobranchial muscles is marked by the expression of Lbx1. ad Whole-mount in situ hybridization of S. torazame embryos at stage 27.5. a, b Expression of Lbx2 in ventral (a) and left lateral (b) views. c, d Expression of Lbx1 in ventral (c) and left lateral (d) views. Arrows show the expression in the anterior extremity of HBM primordium. eg” Transverse sections of a stage 29 embryo at the levels indicated in h (ventral view stained with MyHC antibody). e’g’ The enlarged views of the areas marked in eg. f” and g” are the adjacent sections to f’ and g’, respectively, hybridized with different probes. e’ Lbx1 is expressed in the medial HBM precursor cells (arrowhead) located dorsal to the hyoid arch-derived muscles (double arrowheads). f’, f” Lbx1 is expressed in the medial HBM precursor cells, whereas Lbx2 expression is restricted in the bilateral HBM primordium (f”). g’, g” Earliest differentiation of HBM occurs in the cells in which Lbx2 is downregulated. i At stage 29.5, the anterior medial part of HBM differentiates as coracomandibularis (cmd) muscle. j At stage 30, the anterior tip of early m. coracoarcualis (cac, originally Lbx2-positive) extended anteriorly, forming coracohyoideus (chy) muscle connecting cac muscle and basihyal cartilage, overlapping laterally with m. coracomandibularis. Coracomandibularis now forms a single medial bundle of muscle fibers that connects the coracoarcualis muscle and the lower jaw. k Meckel’s cartilage expressing Sox9 (asterisk). l, m The cac muscle has four segments corresponding to the adjacent pharyngeal arches (pa3-6). l Ventral view. m Left ventrolateral view. ht, heart; m, mouth. Scale bars, al 0.5 mm; m 0.2 mm

In late embryos, rows of Lbx2-positive cells have differentiated into coracoarcualis (CAC) muscle, the posterior paired domain of HBM (Fig. 4g, g’, h) [34]. CAC myofibers consist of 4 segments each of which corresponding to the posterior pharyngeal arches (Fig. 4l, m; pa3-6), a remarkable similarity to the lamprey HBM (Additional file 1: Fig. S1l). Anatomically, CAC originates at the scapulocoracoid cartilage and inserts to the anterior, medially located HBM (coracomandibularis muscle, CMD; Fig. 4i, j), a morphological orientation consistent with that of the amniote rectus cervicus (sternohyoideus) muscle [11, 34].

Lbx1-positive cells, on the other hand, differentiated later than CAC, giving rise to CMD muscle in the midline, located anterior to the CAC muscle (Fig. 4i, j). Unlike the CAC muscle, the CMD muscle was composed of a long single segment of myofibers and inserted to the Meckel’s cartilage (Fig. 4k, l), reminiscent of mammalian geniohyoideus muscle [34].

It is also noteworthy that the entire HBM primordia, including both Lbx1- and Lbx2-positive cell populations, were stained with the ZO-1 antibody (Additional file 1: Fig. S10). This observation suggests that, in the shark, both the HBM precursor cells and the fin muscle primordia are epithelial in nature, and both remain as a coherent aggregate during the process of extension into the distal parts of the body.

Duplicated gnathostome Lbx genes and complexity of skeletal muscles

These results provide a new scheme for the developmental homology of HBM elements and appendicular muscles of the vertebrates (Fig. 5). The catshark CAC muscle (associated with Lbx2 expression) and the lamprey HBM (associated with Lbx-A expression) are both attached with the ventral ends of pharyngeal muscles and do not fuse in the midline (Fig. 5b, c) [11]. Moreover, catshark CAC and lamprey HBM are also similar with respect to the pattern of myofiber segmentation which corresponds to the adjacent pharyngeal arches (Additional file 1: Fig. S1k and l; Fig. 4m; Fig. 5b, c), suggesting their muscle differentiation is under the influence of pharyngeal embryonic components such as cephalic neural crest cells and the cranial mesoderm cells. On the other hand, Lbx1-positive CMD of the shark, which is homologous to the tetrapod geniohyoideus and genioglossus muscles, seems to be a novel muscular component acquired in gnathostomes (Fig. 5c). CMD-equivalent muscles, as well as the appendicular muscles, are lacking in the cyclostomes, whose HBM is entirely bilateral and segmented in accordance with the pharyngeal arches.

Fig. 5
figure5

Evolutionary scheme of vertebrate skeletal muscles with reference to the embryonic expression of Lbx genes. In the hagfish (a), rectus muscle (m. rect) and anterior oblique muscle (m. decussatus) are the hypobranchial muscle counterpart and derived from Lbx-A-positive ventral cells of the somites. In the lamprey (b), Lbx-A is required in the formation of body wall muscles (bwm, light green) and hypobranchial muscle (HBM, dark green). In gnathostomes (c), Lbx1 (blue) and Lbx2 (green) regulate distinct domains of hypobranchial muscles. Lbx1 functions in the tongue (cmd, m. coracomandibularis in the shark) and appendicular muscles (pfm, pectoral fin muscles) both of which are lacking in cyclostomes. Pharyngeal muscles derived from head mesoderm are shown in orange

Considering expression patterns of Lbx1/Lbx2 genes in the wide variety of Osteichthyans, however, the evolutionary pathway seems more complex. In amphibians, only the Lbx1 gene has been identified in genomic sequences, exhibiting a loss of Lbx2 locus in the amphibian lineage (Additional file 1: Fig. S3) [8, 29]. In Xenopus laevis and direct-developing frog Eleutherodactylus coqui, Lbx1 is expressed in the ventral side of the trunk somites [35, 36]. In Xenopus, these Lbx1-positive somitic cells give rise to the “rectus abdominus” muscle that extends from the ventral edge of the somites and eventually surrounds the abdomen of tadpoles, similarly to the body wall muscles of other vertebrates. Xenopus Lbx1 is also expressed in the limb muscle precursors that appear during the metamorphosis [35]. In zebrafish, both Lbx1b and Lbx2 genes were shown to be involved in hypaxial muscles including pectoral fin muscles [8, 37, 38]. It has been suggested that the primary role of Lbx transcription factors is to control the switch of proliferation/differentiation of the muscle precursor cells [8, 39]. Lbx1 and Lbx2 have been suggested to possess overlapping regulatory functions, as the forced expression of Lbx2 could rescue Lbx1 deficiency [8]. Although only limited information about downstream factors of Lbx is currently available [40], the comparative insights shown here suggest that skeletal muscles of vertebrate clades have deployed different combinations of Lbx1 and Lbx2 to ensure differentiation of complex musculature at variable timing of development.

Conclusions

Our results indicate that Lbx1-positive muscle precursors in the gnathostome ancestor would have been acquired to give rise to the novel, distally located skeletal muscles, i.e., the muscles associated with paired appendages and the anterior internalized tongue (Fig. 5). On the other hand, the posterior portion of the HBM as well as the body wall muscles might represent hypaxial muscle having a deeper evolutionary origin that can be traced back to the common ancestor of vertebrates. Our results lead us to propose a new evolutionary hypothesis—namely, that HBMs, the developmental background of which has long been assumed to be similar to that of limb muscles, may have a closer evolutionary relationship with the abdominal muscle that extensively surrounds the trunk coelom, and that the morphological elaboration of HBMs would have been coupled with the functionalization of duplicated Lbx genes.

Materials and methods

Obtaining embryos of lamprey, hagfish, and catshark

Mature adults of the Japanese lamprey L. camtschaticum, the hagfish E. burgeri, and the cloudy catshark S. torazame were collected in Hokkaido, Shimane, and Ibaraki prefectures in Japan, respectively. Embryos of each animal were obtained as previously described [41]. Briefly, lamprey eggs were inseminated in vitro and reared at 9°, followed by embryonic staging according to Tahara [20]. The larvae were further cultured in mineral water as described in Higuchi et al. [41] until they reach 50 mm in body length. Hagfish embryos were collected from the sea floor and incubated in artificial sea water, followed by staging according to Dean [42]. Catshark embryos were laid in the fish tank and staged as described previously [43, 44]. Embryos were fixed in 4% paraformaldehyde or Serra’s fixative. The experiments were conducted according to the institutional and national guidelines for animal ethics, approved by the RIKEN Animal Experiments Committee.

Identification of lamprey and catshark genes

Although we had previously reported partial mRNA sequence of LjLbx-A [10], we searched for the full-length sequence with reference to the genomic sequence [45]. A cDNA fragment covering the putative N-terminal Met and the stop codon was obtained. We replaced the previously registered LjLbx-A sequence with a new complete cDNA sequence under the same GenBank reference number (HM116241). The mRNA sequence of E. burgeri Lbx-A (LC506433) was predicted on the Ensemble Genome Database (transcript ID: ENSEBUT00000001721.1; http://www.ensembl.org) and amplified from embryonic total RNA. We performed a search for genes of the catshark S. torazame (Lbx1, LC506430; Lbx2, LC506431; Sox9, LC506432) using the sequence archive Squalomix (https://transcriptome.riken.jp/squalomix/) containing the products of whole genome sequencing [46]. The corresponding cDNAs were amplified from poly-A RNA of stage 24-30 embryos.

Phylogenetic analysis

Full-length amino acid sequences (summarized in Additional file 2: Table S1) were aligned and phylogenetic trees were constructed by the neighbor-joining method [47] using ClustalX software (http://www.clustal.org) [48]. Positions with gaps were excluded from the analysis. The length of the branches is proportional to the phylogenetic distances estimated using Kimura’s empirical method for protein distances [49]. The scale bar indicates an evolutionary distance of 0.05 amino acid substitution per position in the sequence. The degree of support for internal branches of the tree was assessed in 1000 bootstrap replicates [50].

Immunohistochemistry

To visualize differentiated muscles and neurons, we used the primary antibodies MF20 or A4.1025 (DSHB, University of Iowa) and anti-acetylated tubulin (T6793; Sigma-Aldrich). ZO-1 (61-7300; Thermo Fisher Scientific) was used to detect tight junctions. The samples were subsequently reacted with the secondary antibody, the F(ab’) fragment of goat anti-mouse IgG (H + L) conjugated with horseradish peroxidase (Thermo Fisher Scientific). Sections were then counterstained with either hematoxylin or DAPI.

In situ hybridization

Whole-mount and section in situ hybridization of lamprey, hagfish, and catshark embryos was performed as previously described [10, 41]. In brief, paraffin-wax-embedded sections of embryos were deparaffinized, treated with proteinase K, and hybridized with DIG-labeled RNA probe overnight. Hybridized probes were detected with anti-DIG-AP Fab fragments and visualized with reaction with BM purple AP substrate (11442074001; Roche). Sections were counterstained with Nuclear Fast Red (H-2403; Vector Laboratories). The probe sequence of LjLbx-A is highlighted in Additional file 1: Fig. S2. The probe template for EbLbx-A was amplified with the primers 5′-CGCCCTGGAGGAACTCGCGAG-3′ and 5′-CATTGCCCTTAGCGTAAAGCF-3′. For the catshark, to distinguish the expression of Lbx1 and Lbx2, probes were designed to include the regions highly diverged between the two genes. Primers used to amplify the probe templates were Lbx1, 5′-GGACCTGGAGGAGATGAAGG-3′ and 5′-GACATGCGATGCAACAAGG-3′; Lbx2, 5′-CGAAGGGACTATTCCTTCTCT–3′ and 5′-AGTCCCACCCCTTCCCCAACAA-3′.

Knock-down experiment of lamprey LjLbx-A gene

Fertilized eggs of the lamprey were microinjected at the 1-cell stage with a mixture of Cas9 protein (0.1 ng/nl, PNA Bio) and guide RNA (gRNA, 25 pg/nl) dissolved in PBS. At appropriate stages, the posterior tail of each embryo was amputated and processed for genomic DNA extraction and PCR amplification for the LjLbx-A locus (Additional file 1: Fig. S5). The anterior body part of each embryo was fixed in 4% PFA or Serra’s fixative. After the genomic analyses, individuals with a high deletion rate were examined for phenotypes. As experimental controls, uninjected embryos, embryos injected with Cas9 only, and injected embryos with a low deletion rate were also analyzed and compared (Additional file 1: Fig. S8).

Library preparation for the screening of CRISPR/Cas9-induced mutants by next-generation sequencing

Each embryo was analyzed for the presence or absence of mutations in the LjLbx-A genomic locus by targeted PCR amplification followed by sequencing with Illumina MiSeq. We followed the previously described procedure [51] with modifications. To increase the number of reads and the quality of reads compared to the original protocol, we removed the self-complementary sequence region from one end of the PCR products before the Illumina library preparation (Additional file 1: Fig. S5). The first PCR was performed with 22 cycles using 10 ng of a template DNA extracted from each embryo, with a gene-specific primer containing a 16-nt-long head sequence (head-GS primers; 5′- GCTATGCGCGAGCTGCgtcgagatggactcgctatt-3′ and 5′- GCTATGCGCGAGCTGCgcacgcacgccgggcgacat-3′; Additional file 1: Fig. S2), and the KAPA HiFi HotStart ReadyMix (KAPA Biosystems). Products of each reaction were purified using the AMPureXP beads (Beckman Coulter). The second PCR was performed with 18 cycles, using the full volume of DNA amplified in the first PCR, a head primer containing an 8-nt-long barcode sequence (barcode-head primer; Additional file 3: Table S2), and the KAPA HiFi HotStart ReadyMix. Products of each reaction were purified using AMPureXP beads, quantitated with the Qubit dsDNA HS Assay kit (ThermoFisher Scientific), and combined. Annealing of the GS primer was performed by adding a 200-fold molar amount of the primer to the combined PCR products of 20 ng in a reaction mixture of 24 μl containing 1x ThermoPol Reaction Buffer (NEB), 6 mM MgSO4, and 1.4 mM dNTP mix, followed by incubation at 95 °C for 1 min, 60 °C for 1 min, and snap-cooling on ice. Primer extension was performed by adding 1 μl (8 U) of the Bst DNA polymerase (NEB) to the reaction mixture, followed by incubation at 65 °C for 3 min and 80 °C for 20 min, and snap-cooling on ice. The combined PCR product, after the primer extension, was purified using AMPureXP beads, eluted in 10 μl of EB buffer (Qiagen), and further treated with 36 U of S1 nuclease (Takara) in a reaction mixture of 20 μl containing 1x S1 nuclease buffer at 23 °C for 15 min. The reaction was terminated by adding 0.5 μl of 0.5 M EDTA solution, and the DNA was purified using the AMPureXP beads and eluted in 10 μl of buffer EB. The combined PCR product after primer extension and digestion of the single-stranded region was analyzed by TapeStation (Agilent) to confirm the shortened length of the head and the barcode sequences (24 nt) before Illumina library preparation. Library preparation was performed as described previously [52] using 10 ng of the combined PCR product that does not contain the self-complementary region, together with the Illumina TruSeq compatible adapter.

Amplicon sequencing and detection of deletion on target regions

Sequencing was performed using the library prepared above, without the use of the control PhiX library, on Illumina MiSeq with the MiSeq Reagent Nano Kit v2 (Illumina) to obtain 250-nt-long paired-end reads. Quality control of the sequencing reads was performed using FastQC ver. 0.11.5 (https://www.bioinformatics.babraham.ac.uk/projects/fastqc/). The BBmerge function of BBTools ver. 37.88 [53] was used to merge two overlapping paired reads into a single long read. The merged reads were then trimmed to remove low-quality regions and the Illumina adapter sequences using Trim galore ver. 0.4.2 (https://www.bioinformatics.babraham.ac.uk/projects/trim_galore/). After separating the amplicon reads according to the barcode sequence for each individual (Additional file 3: Table S2), Cutadapt ver. 1.8.3 [54] was used to remove the barcode sequence and the head sequence. The trimmed reads were aligned with the cDNA sequence of LjLbx-A by BBMap of BBTools, and deletion profiles of the CRISPR/Cas9 target sites were visualized and evaluated with the UCSC Integrative Genomics Viewer (IGV) ver. 2.7.2 [55]. The sequencing data have been deposited to the DNA Data Bank of Japan (DDBJ) under the accession number DRA009475.

Availability of data and materials

Newly sequenced genes have been registered in GenBank under the reference numbers shown in the “Materials and methods” section. The amplicon sequencing data of CRISPR/Cas9 experiments have been deposited to the DNA Data Bank of Japan (DDBJ) under the accession number DRA009475 [56]. DNA sequences used in the phylogenetic analyses are listed in Additional file 2: Table S1.

References

  1. 1.

    Mackenzie S, Walsh FS, Graham A. Migration of hypoglossal myoblast precursors. Dev Dyn. 1998;213(4):349–58.

    CAS  PubMed  Google Scholar 

  2. 2.

    Kuratani S. Spatial distribution of postotic crest cells defines the head/trunk interface of the vertebrate body: embryological interpretation of peripheral nerve morphology and evolution of the vertebrate head. Anat Embryol (Berl). 1997;195(1):1–13.

    CAS  Google Scholar 

  3. 3.

    Christ B, Ordahl CP. Early stages of chick somite development. Anat Embryol (Berl). 1995;191(5):381–96.

    CAS  Google Scholar 

  4. 4.

    Dietrich S, Schubert FR, Healy C, Sharpe PT, Lumsden A. Specification of the hypaxial musculature. Development. 1998;125(12):2235–49.

    CAS  PubMed  Google Scholar 

  5. 5.

    Brohmann H, Jagla K, Birchmeier C. The role of Lbx1 in migration of muscle precursor cells. Development. 2000;127(2):437–45.

    CAS  PubMed  Google Scholar 

  6. 6.

    Gross MK, Moran-Rivard L, Velasquez T, Nakatsu MN, Jagla K, Goulding M. Lbx1 is required for muscle precursor migration along a lateral pathway into the limb. Development. 2000;127(2):413–24.

    CAS  PubMed  Google Scholar 

  7. 7.

    Chen F, Liu KC, Epstein JA. Lbx2, a novel murine homeobox gene related to the Drosophila ladybird genes is expressed in the developing urogenital system, eye and brain. Mech Dev. 1999;84(1–2):181–4.

    CAS  PubMed  Google Scholar 

  8. 8.

    Wotton KR, Schubert FR, Dietrich S. Hypaxial muscle: controversial classification and controversial data? Results Probl Cell Differ. 2015;56:25–48.

    CAS  PubMed  Google Scholar 

  9. 9.

    Wei K, Chen J, Akrami K, Sekhon R, Chen F. Generation of mice deficient for Lbx2, a gene expressed in the urogenital system, nervous system, and Pax3 dependent tissues. Genesis. 2007;45(6):361–8.

    CAS  PubMed  Google Scholar 

  10. 10.

    Kusakabe R, Kuraku S, Kuratani S. Expression and interaction of muscle-related genes in the lamprey imply the evolutionary scenario for vertebrate skeletal muscle, in association with the acquisition of the neck and fins. Dev Biol. 2011;350(1):217–27.

    CAS  PubMed  Google Scholar 

  11. 11.

    Adachi N, Pascual-Anaya J, Hirai T, Higuchi S, Kuratani S. Development of hypobranchial muscles with special reference to the evolution of the vertebrate neck. Zoological letters. 2018;4:5.

    PubMed  PubMed Central  Google Scholar 

  12. 12.

    Green SA, Uy BR, Bronner ME. Ancient evolutionary origin of vertebrate enteric neurons from trunk-derived neural crest. Nature. 2017;544(7648):88–91.

    CAS  PubMed  PubMed Central  Google Scholar 

  13. 13.

    Parker HJ, Bronner ME, Krumlauf R. A Hox regulatory network of hindbrain segmentation is conserved to the base of vertebrates. Nature. 2014;514(7523):490–3.

    CAS  PubMed  PubMed Central  Google Scholar 

  14. 14.

    Kuratani S, Kuraku S, Murakami Y. Lamprey as an evo-devo model: lessons from comparative embryology and molecular phylogenetics. Genesis. 2002;34(3):175–83.

    CAS  PubMed  Google Scholar 

  15. 15.

    Kusakabe R, Kuratani S. Evolutionary perspectives from development of mesodermal components in the lamprey. Dev Dyn. 2007;236(9):2410–20.

    CAS  PubMed  Google Scholar 

  16. 16.

    Peters A, Mackay B. The structure and innervation of the myotomes of the lamprey. J Anat. 1961;95:575–85.

    CAS  PubMed  PubMed Central  Google Scholar 

  17. 17.

    Oisi Y, Fujimoto S, Ota KG, Kuratani S. On the peculiar morphology and development of the hypoglossal, glossopharyngeal and vagus nerves and hypobranchial muscles in the hagfish. Zoological Lett. 2015;1:6.

    PubMed  PubMed Central  Google Scholar 

  18. 18.

    Kuratani S, Ueki T, Aizawa S, Hirano S. Peripheral development of cranial nerves in a cyclostome, Lampetra japonica: morphological distribution of nerve branches and the vertebrate body plan. J Comp Neurol. 1997;384(4):483–500.

    CAS  PubMed  Google Scholar 

  19. 19.

    Higashiyama H, Hirasawa T, Oisi Y, Sugahara F, Hyodo S, Kanai Y, Kuratani S. On the vagal cardiac nerves, with special reference to the early evolution of the head-trunk interface. J Morphol. 2016;277(9):1146–58.

    PubMed  Google Scholar 

  20. 20.

    Tahara Y. Normal stages of development in the lamprey, Lampetra reissneri (Dybowski). Zool Sci. 1988;5:109–18.

    Google Scholar 

  21. 21.

    Horigome N, Myojin M, Ueki T, Hirano S, Aizawa S, Kuratani S. Development of cephalic neural crest cells in embryos of Lampetra japonica, with special reference to the evolution of the jaw. Dev Biol. 1999;207(2):287–308.

    CAS  PubMed  Google Scholar 

  22. 22.

    Kusakabe R, Takechi M, Tochinai S, Kuratani S. Lamprey contractile protein genes mark different populations of skeletal muscles during development. J Exp Zoolog B Mol Dev Evol. 2004;302(2):121–33.

    Google Scholar 

  23. 23.

    Kusakabe R, Kuratani S. Evolution and developmental patterning of the vertebrate skeletal muscles: perspectives from the lamprey. Dev Dyn. 2005;234(4):824–34.

    PubMed  Google Scholar 

  24. 24.

    Chen F, Collin GB, Liu KC, Beier DR, Eccles M, Nishina PM, Moshang T, Epstein JA. Characterization of the murine Lbx2 promoter, identification of the human homologue, and evaluation as a candidate for Alström syndrome. Genomics. 2001;74(2):219–27.

    CAS  PubMed  Google Scholar 

  25. 25.

    Letelier J, de la Calle-Mustienes E, Pieretti J, Naranjo S, Maeso I, Nakamura T, Pascual-Anaya J, Shubin NH, Schneider I, Martinez-Morales JR, et al. A conserved Shh cis-regulatory module highlights a common developmental origin of unpaired and paired fins. Nat Genet. 2018;50(4):504–9.

    CAS  PubMed  PubMed Central  Google Scholar 

  26. 26.

    Jagla K, Dolle P, Mattei MG, Jagla T, Schuhbaur B, Dretzen G, Bellard F, Bellard M. Mouse Lbx1 and human LBX1 define a novel mammalian homeobox gene family related to the Drosophila lady bird genes. Mech Dev. 1995;53(3):345–56.

    CAS  PubMed  Google Scholar 

  27. 27.

    Okamoto E, Kusakabe R, Kuraku S, Hyodo S, Robert-Moreno A, Onimaru K, Sharpe J, Kuratani S, Tanaka M. Migratory appendicular muscles precursor cells in the common ancestor to all vertebrates. Nat Ecol Evol. 2017;1(11):1731–6.

    PubMed  Google Scholar 

  28. 28.

    Turner N, Mikalauskaite D, Barone K, Flaherty K, Senevirathne G, Adachi N, Shubin NH, Nakamura T. The evolutionary origins and diversity of the neuromuscular system of paired appendages in batoids. Proc Biol Sci. 2019;286(1914):20191571.

    CAS  PubMed  Google Scholar 

  29. 29.

    Wotton KR, Weierud FK, Dietrich S, Lewis KE. Comparative genomics of Lbx loci reveals conservation of identical Lbx ohnologs in bony vertebrates. BMC Evol Biol. 2008;8:171.

    PubMed  PubMed Central  Google Scholar 

  30. 30.

    Haines L, Currie PD. Morphogenesis and evolution of vertebrate appendicular muscle. J Anat. 2001;199(Pt 1–2):205–9.

    CAS  PubMed  PubMed Central  Google Scholar 

  31. 31.

    Goodrich ES. Studies on the structure and development of vertebrates; 1930.

    Google Scholar 

  32. 32.

    Bultje RS, Castaneda-Castellanos DR, Jan LY, Jan Y-N, Kriegstein AR, Shi S-H. Mammalian Par3 regulates progenitor cell asymmetric division via notch signaling in the developing neocortex. Neuron. 2009;63(2):189–202.

    CAS  PubMed  PubMed Central  Google Scholar 

  33. 33.

    Mayeuf-Louchart A, Montarras D, Bodin C, Kume T, Vincent SD, Buckingham M. Endothelial cell specification in the somite is compromised in Pax3-positive progenitors of Foxc1/2 conditional mutants, with loss of forelimb myogenesis. Development. 2016;143(5):872–9.

    CAS  PubMed  PubMed Central  Google Scholar 

  34. 34.

    Ziermann JM, Freitas R, Diogo R. Muscle development in the shark Scyliorhinus canicula: implications for the evolution of the gnathostome head and paired appendage musculature. Front Zool. 2017;14:31.

    PubMed  PubMed Central  Google Scholar 

  35. 35.

    Martin BL, Harland RM. A novel role for lbx1 in Xenopus hypaxial myogenesis. Development. 2006;133(2):195–208.

    CAS  PubMed  Google Scholar 

  36. 36.

    Sabo MC, Nath K, Elinson RP. Lbx1 expression and frog limb development. Dev Genes Evol. 2009;219(11–12):609–12.

    CAS  PubMed  Google Scholar 

  37. 37.

    Ochi H, Westerfield M. Lbx2 regulates formation of myofibrils. BMC Dev Biol. 2009;9:13.

    PubMed  PubMed Central  Google Scholar 

  38. 38.

    Sagarin KA, Redgrave AC, Mosimann C, Burke AC, Devoto SH. Anterior trunk muscle shows mix of axial and appendicular developmental patterns. Dev Dyn. 2019;248(10):961–8.

    PubMed  Google Scholar 

  39. 39.

    Watanabe S, Kondo S, Hayasaka M, Hanaoka K. Functional analysis of homeodomain-containing transcription factor Lbx1 in satellite cells of mouse skeletal muscle. J Cell Sci. 2007;120(Pt 23):4178–87.

    CAS  PubMed  Google Scholar 

  40. 40.

    Guo L, Yamashita H, Kou I, Takimoto A, Meguro-Horike M, Horike S, Sakuma T, Miura S, Adachi T, Yamamoto T, et al. Functional investigation of a non-coding variant associated with adolescent idiopathic scoliosis in zebrafish: elevated expression of the ladybird homeobox gene causes body axis deformation. PLoS Genet. 2016;12(1):e1005802.

    PubMed  PubMed Central  Google Scholar 

  41. 41.

    Higuchi S, Sugahara F, Pascual-Anaya J, Takagi W, Oisi Y, Kuratani S. Inner ear development in cyclostomes and evolution of the vertebrate semicircular canals. Nature. 2019;565(7739):347–50.

    CAS  PubMed  Google Scholar 

  42. 42.

    Dean B. On the embryology of Bdellostoma stouti. A general account of myxinoid development from the egg and segmentation to hatching. In: Festschrift zum 70ten Geburststag Carl von Kupffer. Gustav Fischer; 1899. p. 220–76.

  43. 43.

    Adachi N, Kuratani S. Development of head and trunk mesoderm in the dogfish, Scyliorhinus torazame: I. embryology and morphology of the head cavities and related structures. Evol Dev. 2012;14(3):234–56.

    PubMed  Google Scholar 

  44. 44.

    Ballard WW, Mellinger J, Lechenault H. A series of normal stages for development of Scyliorhinus-Canicula, the lesser spotted dogfish (Chondrichthyes, Scyliorhinidae). J Exp Zool. 1993;267(3):318–36.

    Google Scholar 

  45. 45.

    Mehta TK, Ravi V, Yamasaki S, Lee AP, Lian MM, Tay BH, Tohari S, Yanai S, Tay A, Brenner S, et al. Evidence for at least six Hox clusters in the Japanese lamprey (Lethenteron japonicum). Proc Natl Acad Sci U S A. 2013;110(40):16044–9.

    CAS  PubMed  PubMed Central  Google Scholar 

  46. 46.

    Hara Y, Yamaguchi K, Onimaru K, Kadota M, Koyanagi M, Keeley SD, Tatsumi K, Tanaka K, Motone F, Kageyama Y, et al. Shark genomes provide insights into elasmobranch evolution and the origin of vertebrates. Nat Ecol Evol. 2018;2(11):1761–71.

    PubMed  Google Scholar 

  47. 47.

    Saitou N, Nei M. The neighbor-joining method: a new method for reconstructing phylogenetic trees. Mol Biol Evol. 1987;4(4):406–25.

    CAS  Google Scholar 

  48. 48.

    Thompson JD, Higgins DG, Gibson TJ. CLUSTAL W: improving the sensitivity of progressive multiple sequence alignment through sequence weighting, position-specific gap penalties and weight matrix choice. Nucleic Acids Res. 1994;22(22):4673–80.

    CAS  PubMed  PubMed Central  Google Scholar 

  49. 49.

    Kimura M. Molecular evolutionary rates contrasted with phenotypic evolutionary rates. In: Kimura M, editor. The neutral theory of molecular evolution. Cambridge: Cambridge University Press; 1983. p. 55–97.

    Google Scholar 

  50. 50.

    Felsenstein J. Confidence limits on phylogenies: an approach using the bootstrap. Evolution. 1985;39(4):783–91.

    Google Scholar 

  51. 51.

    Herbold CW, Pelikan C, Kuzyk O, Hausmann B, Angel R, Berry D, Loy A. A flexible and economical barcoding approach for highly multiplexed amplicon sequencing of diverse target genes. Front Microbiol. 2015;6:731.

    PubMed  PubMed Central  Google Scholar 

  52. 52.

    Kadota M, Hara Y, Tanaka K, Takagi W, Tanegashima C, Nishimura O, Kuraku S. CTCF binding landscape in jawless fish with reference to Hox cluster evolution. Sci Rep. 2017;7(1):4957.

    PubMed  PubMed Central  Google Scholar 

  53. 53.

    Bushnell B, Rood J, Singer E. BBMerge - accurate paired shotgun read merging via overlap. PLoS One. 2017;12(10):e0185056.

    PubMed  PubMed Central  Google Scholar 

  54. 54.

    Martin M. Cutadapt removes adapter sequences from high-throughput sequencing reads. EMBnet J. 2011;17:10–2. https://doi.org/10.14806/ej.17.1.200.

  55. 55.

    Thorvaldsdottir H, Robinson JT, Mesirov JP. Integrative Genomics Viewer (IGV): high-performance genomics data visualization and exploration. Brief Bioinform. 2013;14(2):178–92.

    CAS  PubMed  Google Scholar 

  56. 56.

    Kusakabe R, Higuchi S, Tanaka M, Kadota M, Nishimura O, Kuratani S. Novel developmental bases for the evolution of hypobranchial muscles in vertebrates. Supplementary Datasets. 2020. DDBJ accession DRA009475: https://ddbj.nig.ac.jp/DRASearch/submission?acc=DRA009475.

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Acknowledgements

We thank Drs. Shigehiro Kuraku, Wataru Takagi, and Fumiaki Sugaraha for their valuable input on the genomic and morphological analyses, and Yayoi Nakai and Shunya Kuroda for technical assistances. We also thank Chiharu Tanegashima of the Laboratory for Phyloinformatics, RIKEN BDR, for the library preparation and MiSeq operation.

Funding

This work has been funded by Grant-in-Aid for Scientific Research (C) (19K06683) and Takeda Science Foundation to R.K. and Grant-in-Aid for Scientific Research on Innovative Areas (Research in a Proposed Research Area) (17H06385) to S.K.

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Contributions

R.K., S.H, M.K., and S.K. conceived the project, designed the experiments, and wrote the paper. R.K., S.H., M.T., and O.N. performed the experiments. All authors analyzed and discussed the data. All authors approved the final version of the manuscript.

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Correspondence to Rie Kusakabe.

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Supplementary information

Additional file 1: Figures. S1-S10.

Skeletal muscle formation during lamprey embryogenesis (Fig. S1). Genomic structure of LjLbx-A gene and positions of CRISPR/Cas9 targets (Fig. S2). Phylogenetic analysis of the cyclostome and catshark Lbx genes (Fig. S3). Expression of LjLbx-A in the dorsal median fin muscle primordia (Fig. S4). Workflow and additional data for lamprey genome editing experiments (Fig. S5-S8). Expression of catshark Lbx2 in the extending HBM precursor cells (Fig. S9). ZO-1 staining of HBM primordium in the catshark embryo (Fig. S10).

Additional file 2: Table S1.

Lbx genes compared in this study.

Additional file 3: Table S2.

Barcode primers used in lamprey genome editing experiments.

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Kusakabe, R., Higuchi, S., Tanaka, M. et al. Novel developmental bases for the evolution of hypobranchial muscles in vertebrates. BMC Biol 18, 120 (2020). https://doi.org/10.1186/s12915-020-00851-y

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Keywords

  • Hypobranchial muscle
  • Development
  • Lamprey
  • Hagfish
  • Shark
  • Skeletal muscle
  • Lbx genes
  • Evolution
  • Vertebrates