Skip to main content

Thank you for visiting nature.com. You are using a browser version with limited support for CSS. To obtain the best experience, we recommend you use a more up to date browser (or turn off compatibility mode in Internet Explorer). In the meantime, to ensure continued support, we are displaying the site without styles and JavaScript.

Molecular ontogeny of the stomach in the catshark Scyliorhinus canicula

Abstract

The origin of extracellular digestion in metazoans was accompanied by structural and physiological alterations of the gut. These adaptations culminated in the differentiation of a novel digestive structure in jawed vertebrates, the stomach. Specific endoderm/mesenchyme signalling is required for stomach differentiation, involving the growth and transcription factors: 1) Shh and Bmp4, required for stomach outgrowth; 2) Barx1, Sfrps and Sox2, required for gastric epithelium development and 3) Cdx1 and Cdx2, involved in intestinal versus gastric identity. Thus, modulation of endoderm/mesenchyme signalling emerges as a plausible mechanism linked to the origin of the stomach. In order to gain insight into the ancient mechanisms capable of generating this structure in jawed vertebrates, we characterised the development of the gut in the catshark Scyliorhinus canicula. As chondrichthyans, these animals retained plesiomorphic features of jawed vertebrates, including a well-differentiated stomach. We identified a clear molecular regionalization of their embryonic gut, characterised by the expression of barx1 and sox2 in the prospective stomach region and expression of cdx1 and cdx2 in the prospective intestine. Furthermore, we show that gastric gland development occurs close to hatching, accompanied by the onset of gastric proton pump activity. Our findings favour a scenario in which the developmental mechanisms involved in the origin of the stomach were present in the common ancestor of chondrichthyans and osteichthyans.

Introduction

The origin of specialised digestive structures is considered a major step in the evolution of life1. This event predated the origin of metazoans, when eukaryotic cells became predatory, capturing and accumulating food in vacuoles by phagocytosis2. However, the formation of a tight epithelium surrounding a digestive canal, which made possible the articulation between extracellular and intracellular digestion, was then a decisive evolutionary step for metazoans1,3,4. This epithelial layer, derived from the embryonic endoderm, has been evolving for approximately 700 million years5, and gave rise to the highly complex gastrointestinal tract (GIT) found in jawed vertebrates.

The morphological changes that took place during the evolution of the GIT in these organisms include a marked antero-posterior morphological regionalization and the emergence of new cell types, adapting each compartment to a specific function during food digestion. In this context, a novel anatomical structure emerged, housing 11 distinct cell types embedded within deep pits and contiguous glandular structures — the stomach6,7.

The absence of a stomach-like structure in lineages that diverged prior to the origin of jawed vertebrates suggests that this structure originated during gnathostome evolution8. Yet, the limited information regarding the internal anatomy of vertebrate fossils makes the transition between a morphologically unregionalized into a regionalized GIT unclear. Within the chondrichthyans, the Holocephali (chimaeras) are stomach-less and their genomes lack genes involved in acid-peptic digestion8,9. In contrast, the elasmobranchs (sharks, skates and rays) do have an acid-peptic stomach with gastric glands8,10,11. Moreover, their genomes contain the elements responsible for the gastric function, the genes encoding the H+/K+ ATPase α and β subunits (atp4a, atp4b) and the genes encoding pepsinogens8,11,12. These features appear to be conserved in most lineages of osteichthyans, the sister group of chondrichthyans. Nevertheless, secondary reduction or loss of stomach structures appears to have occurred in multiple teleost species, dipnoids and monotremes8,12,13.

A critical gap in our understanding of GIT evolution concerns the molecular networks that facilitated differentiation of the GIT into functionally distinct sections during the vertebrate radiation. Previous data (mostly from amphibian, avian and mammalian development) show that the GIT is formed from an embryonic tubular structure, which then compartmentalizes into a foregut, midgut and hindgut14,15. This process is preceded by differential gene expression along the antero-posterior axis, which is decisive in allowing alternative paths in GIT differentiation16. Thus, acquisition or up-regulation of particular genes may have triggered the antero-posterior regionalization of the GIT during evolution. Proteins encoded by genes such as Shh (Sonic hedgehog), Bmp4 (Bone morphogenetic protein 4), Fgf10 (Fibroblast growth factor 10), Barx1 (BarH-like homeobox 1), Sox2 (Sex determining region Y-box 2), Cdx1 (Caudal type homeobox 1) and Cdx2 (Caudal type homeobox 2) have distinct roles in the definition of a gastric versus an intestinal phenotype16,17,18,19,20. The Shh protein is produced within the gut endoderm and triggers the expression of Bmp4 in the adjacent midgut and hindgut mesenchyme. Bmp4 proteins then reduce the mesodermal growth in these non-stomach regions, allowing the enlargement of this tissue exclusively in the foregut21. In contrast, Fgf10 protein is typically a mesenchymal factor that acts on the endodermal layer, strongly impacting epithelial elaboration during intestinal development22.

Expression of Barx1 in the posterior foregut, the prospective stomach region, is essential for the differentiation of the gastric epithelium. Barx1 inhibits Wnt signalling (Wingless-related integration site proteins), which operates in the uncommitted endoderm through regulation of Sfrps (Secreted frizzled-related proteins) that are Wnt antagonists23. Lack of Wnt signalling inhibition within the gut endodermal cells leads them to differentiate into intestinal epithelial cells23,24. In addition, Sox2 seems to have a pivotal role in generating morphologically and physiologically distinct epithelial cell types in the foregut and midgut, contributing to the formation of the gastric glands20. Finally, Cdx1 and Cdx2 are involved in the early patterning and maintenance of the intestinal epithelium25.

How and when these molecular interactions became active, during vertebrate GIT evolution, remain largely unexplored. Here we provide an extensive characterization of the GIT development in the shark model Scyliorhinus canicula, with the aim of identifying the ancient molecular mechanisms involved in the origin of the stomach. As elasmobranchs, S. canicula represents the chondrichthyan lineage with an unequivocal stomach, which seems to be a plesiomorphic feature of jawed vertebrates9,26. Overall, these results demonstrate profound conservation of the molecular mechanisms of GIT development in sharks, suggesting that the origin of the stomach involved the assembly of molecular networks that predate the divergence of chondrichthyans and osteichthyans.

Results

Development and activation of the gastric function in S. canicula

A radial enlargement of the posterior foregut segment, characterized by a stratified epithelium, marks the initiation of stomach development in S. canicula at st.24 (Fig. 1A,B). Within this region, acid mucins are detected by AB-PAS staining in a thin layer under the epithelium from st.24 to 28 (Fig. 1A–D) and then spread throughout the mesenchymal tissue (Fig. 1E,F). Basic mucins, in contrast, are detectable in the epithelial layer contacting the lumen between st.26 and st.32 (Fig. 1C–J), suggesting that mucus production starts before the onset of gastric gland formation. Differentiation of the spiral intestine is detectable posterior to the developing stomach between st.23 and st.32, closely resembling other descriptions for elasmobranchs27,28,29.

Figure 1
figure1

Stomach development in S. canicula. Alcian-Blue-PAS staining performed in histological sections of S. canicula at st.24 (A,B), 28 (C,D), 29 (E,F), 31 (G,H) and 32 (I,J). Right panels show higher magnifications of the prospective stomach depicted in the adjacent left panel (boxed). (A,B,E) and (F) are sagittal sections and (C,D), (GJ) are coronal sections. (bmc): basic mucins; (ep1): single epithelial layer; (ep2): stratified epithelium; (es): oesophagus; (ey): eye; (fb): forebrain; (hb): hindbrain; (hmc): acid mucins; (ht): heart; (int): intestine; (liv): liver; (lu): lumen; (m): mouth; (mb): midbrain; (mes): mesenchyme; (nc): notochord; (np): nasal pit; (nt): neural tube; (ov): otic vesicle; (p): pancreas; (ph): pharyngeal arches; (st): stomach; (sv): spiral valve. (A,B) Initiation of gastric differentiation at st.24. Single epithelial layer (ep1) in the oesophagus (es) contrasting with stratified epithelium (ep2) in the prospective stomach (st). Layer of acid mucins (hmc) between the mesenchyme (mes) and the epithelium. (C,D) Gastric enlargement (st) at st.28. Layer of basic mucins detectable in the epithelium surface contacting with the lumen (lu). (E,F) Thickening of the epithelial and mesenchymal layers forming the stomach (st) at st.29. Mesenchymal layer with cells surrounded by acid mucins (hmc). (G,H) Stomach positioning between the liver lobes (li) and adjacent to the pancreas (p) at st.31. (I,J) Mesenchyme layer forming differentiated domains with apparent distinct levels of acid mucins at st.32. Inserted panel in J shows additional detail of the gastric epithelium and adjacent mesenchyme. Scale bars: (A,C,E,G), I-1000 µm; (B,D,H)-100 µm; F-200 µm; J-50 µm.

By st.33, cyto-differentiation of the stomach region leads to the formation of cell layers that typically characterize this structure in humans30. The mucosa is formed by a thick folded epithelium adjacent to mesenchyme and a thin layer of smooth longitudinal and circular smooth muscle (Fig. 2A). The submucosa is composed of undifferentiated connective tissue and the serosa appears as a thin layer of epithelial tissue. As in earlier stages, a thin layer of basic mucins is detected at the luminal surface of the developing stomach. However, the gastric proton pump (H+/K+ATPase) is not yet present, as there is no positive immunoreactivity with the C2 antibody against the catalytic subunit (Fig. 2B). Moreover, no zymogen granules are detected using fluorescent eosin staining (Fig. 2C), which would indicate the presence of pepsinogens31. However, gene expression analyses revealed that the genes encoding the catalytic α-subunit (atp4a) and the non-catalytic β-subunit (atp4b) of H+/K+ATPase are expressed in the epithelium of the prospective stomach from st.27 onwards (Fig. 3A,B), suggesting that the events that culminate with the assembly of the heterodimeric proton pump H+/K+ATPase start before the activation of the gastric function.

Figure 2
figure2

Activation of the gastric function in S. canicula. Histological sections in the stomach region of S. canicula, from st.33 to adulthood. (bmc): basic mucins; (epi): epithelial layer; (gg): gastric glands; (gp): gastric pits; (mes): mesenchyme; (mu): mucosa; (mc) mucous cells; (nk): neck cells; (sm): submucosa. (AD) Alcian-Blue-PAS staining performed on (A). Production of basic mucins (bmc) and presence of distinct layers at st.33 such as the mucosa (mu) and submucosa (sm). The mucosa (mu) is formed by epithelial (epi) and mesenchymal layers (mes). (B) Detection of gastric glands (gg) and mucus producing cells from st.34. Note neck cells (nk) and surface foveolar cells or mucous cells (mc) close to the lumen. (C). Well-demarked gastric pit (gp) in one day post-hatching sections (Ph1) with mucous cells (mc) at the surface of the epithelium and within the gastric pits (gp). (D) Morphology of the gastric glands during adulthood showing mucous cells (mc) within the gastric pits (gp) and visible lumens in the gastric glands (gg). (EH) Immunoreactivity of the C2 antibody detecting the gastric pump. H+/K+-ATPase (Atp4a, in green) identified from st.34 to adulthood within the oxynticopeptic cells of the gastric glands (gg). (IL) Pepsinogen zymogen granules (zm) identified with eosin in the oxynticopeptic cells of the gastric glands (gg), from st.34 to adulthood.

Figure 3
figure3

Onset of gastric function during S. canicula development. Gene expression analyses performed by in situ hybridization (A,B) and qPCR (C,D). (A,B) Developmental stages indicated at the bottom of each panel. In situ hybridizations performed in dissections of the GIT showing expression of atp4a (A) and atp4b (B) in the epithelium of the foregut (fg), located between the lobed-liver (liv). Insert in A shows a transversal section throughout the foregut in which atp4a expression is detected lining the luminal surface of the epithelium (arrowhead). (C,D) Gene expression analyses performed with tissues dissected from the anterior and posterior gastrointestinal tract (GIT), corresponding to the prospective stomach (a) and intestine (p), respectively. Note higher expression of atp4a (C) in the prospective stomach region than in the intestine at st. 33 (*p < 0.05) and then a drastic increase in the expression of this gene and pgc (D) during st.34 (**p < 0.01). Embryos selected as representatives of st.34 were 160–165 days old.

The first sign of gastric proton pump protein expression is detected during st.34, when H+/K+ATPase immunoreactive cells become detectable in the presumptive gastric glands embedded within the glandular mucosa, which extends under a layer of secretory mucous epithelial cells, also known as foveolar cells, filled with basic mucins (Fig. 2D). Mucous neck cells are also found at this stage within the gastric pits (Fig. 2E) and zymogenic cells appear within this glandular mucosa (Fig. 2F). Gene expression analyses reveal that during this stage the expression of genes directly related with the gastric function, such as atp4a and pgc (Pepsinogen C), drastically increase specifically in the prospective stomach region (Fig. 3C,D).

One day after hatching, the foveolar cells, producers of basic mucins, form a layer in contact with the lumen of the stomach and also within the gastric pits (Fig. 2G). The active state of the gastric function is also inferred from the IHC presence of Atp4a and zymogen granules in the prospective gastric tubular glands (Fig. 2H,I). The post hatch gastric mucosa is similar to that of adult catsharks, although the lumen of the gastric glands is further enlarged (Fig. 2J–L). Thus, identification of gastric glands at st.34 indicates that the stomach of S. canicula is prepared for digestion prior to hatching.

Molecular regionalization of the GIT during S. canicula development

To uncover the molecular mechanisms involved in GIT regionalization in chondrichthyans, we carried out gene expression assays in S. canicula for shh, bmp4 and fgf10. We found that shh was expressed throughout the GIT at st.23, while bmp4 expression appeared confined to the midgut and hindgut regions at st.25 (Fig. 4A,B). The same patterns are found in tetrapod embryos, where endodermally secreted Shh is thought to induce Bmp4 production in the underlying mesenchyme of the midgut and hindgut, which leads to the inhibition of growth and sets the conditions for stomach enlargment21,32. In addition, we found fgf10 expression throughout the GIT at st.27 (Fig. 4C), suggesting that fgf10 acts on intestinal development, as demonstrated in osteichthyans22,33,34. Together these data point to a conservation of the epithelial-mesenchymal interactions involved in the regionalization of the GIT in chondrichthyans.

Figure 4
figure4

Molecular regionalization of the stomach during S. canicula development. Gene expression analyses performed by in situ hybridization (A,B,D,E,F) and qPCR (GI) Developmental stages in (A,B,D,E,F) indicated in lower left corner (st.). (GIT): Gastro intestinal tract; (gl) gills; (hg) hindgut; (ht) heart; (int) intestine; (mg) midgut; (nt) neural tube; (ph) pharyngeal arches; (ov) otic vesicle; (sto) stomach, ***proximal region of the yolk stalk. (A,C). Expression of shh (A) bmp4 (B) and fgf10 (C,D) along the GIT between st. 23 and 27. (D) Strong barx1 expression in the prospective stomach (sto), contrasting with the intestinal region (int) at st.30. (E) Initial expression of sfrp2 along the GIT at st. 25 and histological section (E’) showing expression in the dorsal mesenchyme surrounding the GIT (arrows). (F). Expression of sox2 evident in the prospective epithelium of the stomach (sto) shown in a dissection of this organ (left panel) and in a transverse histological section (F’). (GI) Relative expression quantification (2−∆CT), plus standard deviations, for barx1 (G), sfrp2 (H), and sox2 (I). Black and white bars show the expression levels in the anterior (a) and posterior (p) fragments of the GIT throughout development, corresponding respectively to the prospective stomach and intestine. The statistically significant differences found between the anterior and posterior portions of the GIT (T-test) are highlighted with asterisks (*p < 0.05; **p < 0.01). Note higher expression of the three genes in the prospective stomach region than in the intestinal region throughout development.

Considering the involvement of Barx1 in stomach development in osteichthyan models19,23,35, we then asked how far back in evolution the expression of this transcription factor became restricted to the posterior foregut mesenchyme to potentiate the origin of the gastric epithelium. We found that S. canicula barx1 was expressed in the presumptive stomach region throughout development, but was only weakly expressed in the presumptive intestine (Fig. 4D,G). These data suggest that barx1 may also regulate mesenchymal signals involved in the specification of the stomach in chondrichthyans. The expression of sfrp2 was also found within the GIT mesenchyme of S. canicula (Fig. 4E,H). At st.25, sfrp2 expression is detectable along the prospective intestine, particularly in the most dorsal mesenchyme surrounding the gut epithelium (Fig. 4E). However, its expression was significantly higher in the prospective stomach than in the intestine at st.29 and st.31. These results suggest that Sfrps may modulate Wnt signalling during the development of the catshark’s gut, contributing to the generation of the highly polymorphic epithelium found along the GIT, as described in osteichthyan models16,23,36.

In order to analyse whether epithelial signals, which are involved in stomach development in osteichthyans, are also active in chondrichthyans, we studied the expression of sox2 in S. canicula. This transcription factor has been implicated in the differentiation of the gastric epithelium in osteichthyans, namely in its stratification and glandular morphogenesis20. We found higher levels of sox2 expression in the prospective stomach of S. canicula than in the prospective intestine region (Fig. 4F–I), specifically marking the epithelium (Fig. 4F). These results suggest that the sox2 gene is involved in the gastric development not only in osteichthyans, but also in chondrichthyans.

We also investigated the conservation of the molecular mechanisms underlying intestinal development in sharks by examining the expression of genes encoding intestine-specific transcription factors well characterized in osteichthyans18,25,37, cdx1 and cdx2. We found that their expression patterns were restricted to the developing intestinal region of S. canicula (Fig. 5A–D). In this species, cdx1 was detected along the mesenchyme surrounding the hindgut and midgut segments, including in the forming spiral valve, from st.24 (Fig. 5A,B). The cdx2 expression presented much higher levels in the prospective intestine than in the prospective stomach through development (Fig. 5C,D). Taken together, the expression profiles found in S. canicula indicate that the molecular mechanisms involved in GIT regionalization are conserved between osteichthyans and chondrichthyans.

Figure 5
figure5

Molecular regionalization of the intestinal region during S. canicula development. Gene expression analyses performed by in situ hybridization (A,B,D) and qPCR (C). Developmental stages in (A,B,D) indicated in lower right corner. (GIT) gastrointestinal tract; (hg): hindgut; (ht): heart; (ov) otic vesicle; (sv) spiral valve. (A). Expression of cdx1 along the GIT at st.24, including in the spiral valve (sv). (B) Transversal histological section throughout the spiral valve (sv) showing cdx1 expression in the mesenchymal layer (arrows). (C) cdx2 gene expression levels in the GIT throughout development. Black and white bars show the expression levels in the anterior (a) and posterior (p) fragments of the GIT throughout development, corresponding respectively to the prospective stomach and intestine. The statistically significant differences found between the anterior and posterior portions of the GIT (T-test) are highlighted with asterisks (*p < 0.05; **p < 0.01). Note higher expression in the prospective intestinal region than in the stomach region throughout development. (D) Expression of cdx2 detected in the hindgut (hg) at st.25.

Discussion and Conclusion

Gastric gland development and activation in S. canicula

In this study, we characterized the development of the GIT in the catshark S. canicula, identifying the onset of gastric gland formation and evaluating the expression of genes involved in their activation. The emergence of the gastric glands is commonly seen as an indicator of a fully developed stomach38,39. However, gastric glands alone do not determine the complete functionality of the stomach, which also requires pepsin activity to accomplish its digestive function40,41. Here we identified a marked increase of both atp4a and pgc expression at the developmental stage in which gastric glands first appear (st.34), and this is accompanied by the emergence of a layer of active mucous cells facing the lumen of the stomach. These cells function to protect the stomach epithelium against acidity42. Thus, our results clearly suggest that S. canicula hatch with a morphologically functional stomach.

GIT regionalization in S. canicula

Gut development in tetrapods generically involves (1) early endoderm specification, (2) endodermal tube formation, (3) cephalocaudal regionalization forming the foregut, the midgut and the hindgut segments (4) cyto-differentiation within these segments and (5) their functional activation. Endoderm specification was recently characterized in S. canicula at the earliest blastula stages, using the endodermal lineage markers43: gata6, sox17 and hex. In addition, reports on the expression of 5’HoxD genes in this species27,44 identified a molecularly regionalized gut as early as st.22. Both hoxd9 and hoxd10 were detected up to the level of the midgut, while hoxd12 expression was exclusively found in the hindgut region. Later on, at st.25, hoxd13 additionally marks the hindgut region27,44. Similarly, the paralogous hoxa genes were observed in antero-posterior regionalized patterns along the gut anteroposterior axis45. In skates, both hoxa13 and hoxd13 are expressed in the hindgut, where they have been proposed to play an essential role in colon specification46. Thus, cephalocaudal molecular regionalization of the chondrichthyan gut involves the same genes that are activated in osteichthyans to specify distinct segments with specialized digestive functions.

In addition, our data suggest that the epithelial-mesenchymal signalling interactions, which take place along the antero-posterior GIT and lead to the organogenesis of the stomach in humans30, also appear to be conserved in chondrichthyans. Indeed, we showed that shh and bmp4, which mediate the epithelial-mesenchymal signalling involved in the regionalization of the foregut, midgut and hindgut in osteichthyan model organisms, are both expressed in the developing GIT of S. canicula21,32. Moreover, we found that bmp4 is expressed specifically in the midgut and hindgut regions during the initial enlargement of the stomach in S. canicula. Bmp4 proteins were shown to reduce mesodermal growth within these most posterior regions of the GIT, indirectly causing the enlargement of the stomach anteriorly16,21,32. Our findings raise the hypothesis that activation of Shh-Bmp signalling in the posterior region of the GIT may have been a fundamental step towards the acquisition of the stomach in gnathostomes. Further studies using organisms that retain the pre-gnathostome condition will test the validity of this hypothesis. In addition, bmp4 is expressed, together with shh, throughout the entire GIT during zebrafish development, and this teleost fish fails to develop a distinct stomach with gastric glands47. Therefore, loss of restriction of the bmp4 expression to the posterior portions of the GIT may explain the recurrent stomach loss that occurred in several gnathostome lineages8.

Molecular cues for stomach development in S. canicula

The development of a functional stomach relies on the expression of the homeobox gene barx1, which inhibits the Wnt signalling through Sfrps to prevent the differentiation of an intestinal-like epithelium23. Our data show that in S. canicula, barx1 is highly expressed in the prospective stomach regions, which closely resembles the expression patterns found in mammals and birds16,23,35. Therefore, our data imply that the molecular processes involved in gastric epithelium differentiation are conserved in these chondrichthyans. Paradoxically, in the stomachless zebrafish Danio rerio, barx1 is expressed specifically in the foregut segments48 and several sfrp genes are also expressed in the developing gut36. We hypothesize that the barx1 expression in zebrafish may not be sufficient to trigger the Wnt signalling inhibition needed for a clear specification of a gastric-like epithelium. Interestingly, during stomach development in mice, the Barx1 expression is precisely regulated in space and time by specific microRNAs47, translational regulators that may have been involved in drastic morphological changes that occurred in particular vertebrate lineages49. Thus, further studies investigating barx1 regulation by miRNAs during zebrafish GIT development will be informative to the developmental origin of the stomach and its secondary loss in numerous gnathostome species.

The transcription factor Sox2 has been implicated in antero-posterior specification of the gastric epithelium and, later, in the differentiation of the gastric glands17,18. Moreover, Sox2 expression is sufficient to activate ectopically the foregut transcriptional program, which exerts a dominant effect on intestinal cell fate in mice17. Thus, activation of this gene during evolution might have been essential for the origin of the stomach in vertebrates. Our data show that yet another transcription factor typically involved in the differentiation of the gastric epithelium in mammals17,18,20, sox2, presents a conserved expression pattern in the prospective stomach region of S. canicula. Contrastingly, cdx1 and cdx2 expression is associated with development of the intestinal region, which also resembles the general pattern found in mammals25.

Intriguingly, the agastric zebrafish does have an anteriorly restricted sox2 expression pattern50, suggesting that the expression of this gene is not sufficient to drive the formation of a functional gastric epithelium. As for barx1, we favour an evolutionary scenario in which modulation of sox2 expression levels might have been instrumental in triggering the origin of the gastric epithelium. In fact, sox2 seems to be expressed in a gradient and to have multiple dose-dependent roles during the patterning and differentiation of anterior foregut endoderm51. Thus, changes in this gradient may have caused an alteration in the expression of their downstream targets, which may explain the gut plasticity found in gnathostome lineages.

Overall, our results show that, in catsharks, development of an acid-peptic stomach complete with gastric glands concludes close to hatching, and suggest that the differentiation of the GIT in elasmobranchs and osteichthyans share molecular mechanisms. This involves not only activation of master regulators of stomach and intestine differentiation but also regulation of their expression levels. Addressing the mechanisms that regulate these gene expression patterns and allow for their modulation in different organisms will be essential for understanding the origin of these structures, their absence or loss in certain chondrichthyan and osteichthyan lineages, and their diversification during gnathostome evolution.

Methods

Collection and staging of embryos

Scyliorhinus canicula eggs were obtained from the Roscoff Marine Biological Station (France), Menai Strait (UK) or from locally collected pregnant females kept in tanks in the aquatic bioterium of CIIMAR (Portugal). Embryos were staged according to Ballard and colleagues52, saved in RNALater (Thermo Fisher Scientific) and stored at −80 °C for RNA extraction and cDNA synthesis or fixed in 4% paraformaldehyde in phosphate buffered saline (pH 7.4) for 24 h at 4 °C, dehydrated in a methanol series and stored at −20 °C to be used for in situ hybridizations, immunohistochemistry and histology. All experiments conducted in this study were carried out at Biotério de Organismos Aquáticos (BOGA, CIIMA) aquatic animal facilities and have been approved by the CIIMAR ethical committee and by CIIMAR Managing Animal Welfare Body (ORBEA) according to the European Union Directive 2010/63/EU “on the protection of animals used for scientific purposes”.

Histology and Immunohistochemistry

Histological sections (5 µm) of paraffin-embedded tissues were stained with haematoxylin-eosin (H&E) or Alcian blue (pH 2.5), periodic acid-Schiff (AB-PAS) and haematoxylin. Sections were used to characterize stomach development in S. canicula and detect the presence of acid mucins (blue) and neutral-acidic mucins (magenta). Eosin fluorescence allowed visualization of eosinophilic zymogen granules typically found in the acinar cells of gastric glands31. Immunohistochemistry (IHC), with rabbit polyclonal antibody (C2) against the H+/K+ATPase α - or catalytic subunit (HKα1)53, was used to identify the onset of HKα1 production during S. canicula development. For IHC, deparaffinised sections were rehydrated in TPBS (0.05% tween-20 in Phosphate Buffered Saline, pH 7.4) and blocked with 5% normal goat serum in 1% bovine serum albumin (BSA)/TPBS. They were then incubated with C2 antibody diluted 1:200 in 1% BSA/TPBS overnight at 4 °C. After TPBS washes, slides were incubated in secondary conjugated goat anti-rabbit Alexa Fluor 488 antibody (Invitrogen) diluted 1:500 in 1% BSA/TPBS for 1 hour at 37 °C. Slides were counter stained with DAPI and cover-slipped using a glycerol based fluorescence mounting media (10% mowiol, 40% glycerol, 0.1% 1,4-diazabicyclo[2.2.2]octane (DABCO, Sigma Aldrich), 0.1 M Tris-pH 8.5). Histological and immunohistochemical images were acquired with a respective Leica DFC300FX digital colour camera and Leica DFC 340 FX cooled digital camera mounted on a Leica DM6000 B wide field epi-fluorescence microscope.

Cloning and Quantitative Real-Time PCR experiments

The prospective stomach and intestinal region of S. canicula embryos was dissected, from st.25 to close to hatching. RNA was extracted from these samples (Aurum total RNA kit, BioRad) and converted into cDNA using High Capacity cDNA RT kit (Applied Biosystems). A 2.34 kb partial sequence of atp4a was isolated from a cDNA pool, by Polymerase Chain Reaction (PCR), using degenerate primers previously designed for chondrichthyans8,54. The full-length sequence was obtained with RACE methods (SMARTer RACE Clontech; GeneBank accession KX519315). Reverse transcription-PCR (RT-PCRs) reactions, using degenerate primers, were performed to amplify fragments of bmp4, fgf10, and shh. The DNA fragments amplified were cloned into pDrive vector (Qiagen). Quantitative Real-time PCR reactions (qPCR) were used to evaluate gene expression profiles of atp4a, pgc, barx1, sfrp2, sox2, and cdx2 throughout development, in the prospective stomach and intestinal regions, using iQ Supermix with SYBR Green (Bio-Rad). Relative expression levels were normalized with β-actin2 gene (actb2) expression, shown to be constant throughout S. canicula GIT development, and relative gene expression quantifications were calculated using the 2−ΔCT method55. These analyses were performed with a minimum of three biological replicates per stage, depicted throughout development. The differential expression between the prospective stomach and intestinal region was evaluated statistically using Student’s t-test, p < 0.05 and p < 0.01.

In situ Hybridization (ISH)

Gene expression patterns were evaluated using in situ hybridizations (ISH) following previously established protocols56. RNA probes, labelled with digoxygenin 11 UTP (DIG), were synthetized from a cDNA library constructed in the pSPORT1 vector57 or from PCR amplifications cloned into pDrive vectors.

References

  1. 1.

    Nielson, C. Six major steps in animal evolution: are we derived sponge larvae? Evol Dev 10, 241–257 (2008).

    Article  Google Scholar 

  2. 2.

    De Nooijer, S., Holland, B. R. & Penny, D. The emergence of predators in early life: There was no garden of eden. PloS one 4, https://doi.org/10.1371/journal.pone.0005507 (2009).

  3. 3.

    Yonge, C. M. Evolution and adaptation in the digestive system of the Metazoa. Biol Rev Camb Philos 12, 87–115, https://doi.org/10.1111/J.1469-185x.1937.Tb01223.X (1937).

    Article  Google Scholar 

  4. 4.

    Peterson, K. J., McPeek, M. A. & Evans, D. A. D. Tempo and mode of early animal evolution: inferences from rocks, Hox, and molecular clocks. Paleobiol 31, 36–55, https://doi.org/10.1666/0094-8373(2005)031[0036:Tamoea]2.0.Co;2 (2005).

    Article  Google Scholar 

  5. 5.

    Nielsen, C. Animal evolution: interrelationships of the living phyla. 3rd edition, (Oxford University Press).

  6. 6.

    Karam, S. M., Li, Q. T. & Gordon, J. I. Gastric epithelial morphogenesis in normal and transgenic mice. Am J Physiol-Gastr L 272, G1209–G1220 (1997).

    CAS  Google Scholar 

  7. 7.

    Karam, S. M., Yao, X. B. & Forte, J. G. Functional heterogeneity of parietal cells along the pit-gland axis. Am J Physiol-Gastr L 272, G161–G171 (1997).

    CAS  Google Scholar 

  8. 8.

    Castro, L. F. et al. Recurrent gene loss correlates with the evolution of stomach phenotypes in gnathostome history. Proc Roy Soc. B 281, 20132669, https://doi.org/10.1098/rspb.2013.2669 (2014).

    CAS  Article  Google Scholar 

  9. 9.

    Holmgren, S. & Nilsson, S. In Sharks, Skates, and Rays: The Biology of Elasmobranch Fishes (ed. W. C. Hamlett) 144–173 (The Johns Hopkins University Press, 1999).

  10. 10.

    Michelangeli, F., Ruiz, M. C., Dominguez, M. G. & Parthe, V. Mammalian-like differentiation of gastric cells in the shark Hexanchus griseus. Cell Tissue Res 251, 225–227 (1988).

    CAS  Article  Google Scholar 

  11. 11.

    Nguyen, A. D. et al. Purification and characterization of the main pepsinogen from the shark. Centroscymnus coelolepis. J Biochem 124, 287–293 (1998).

    CAS  PubMed  Google Scholar 

  12. 12.

    Castro, L. F. C., Lopes-Marques, M., Goncalves, O. & Wilson, J. M. The evolution of pepsinogen c genes in vertebrates: duplication, loss and functional diversification. PloS one 7, e32852, https://doi.org/10.1371/journal.pone.0032852 (2012).

    ADS  CAS  Article  PubMed  PubMed Central  Google Scholar 

  13. 13.

    Ordonez, G. R. et al. Loss of genes implicated in gastric function during platypus evolution. Genome Biol 9, R81, https://doi.org/10.1186/gb-2008-9-5-r81 (2008).

    CAS  Article  PubMed  PubMed Central  Google Scholar 

  14. 14.

    Wells, J. M. & Melton, D. A. Vertebrate endoderm development. Ann Rev Cell Dev Biol 15, 393–410, https://doi.org/10.1146/Annurev.Cellbio.15.1.393 (1999).

    CAS  Article  Google Scholar 

  15. 15.

    Smith, D. M., Grasty, R. C., Theodosiou, N. A., Tabin, C. J. & Nascone-Yoder, N. M. Evolutionary relationships between the amphibian, avian, and mammalian stomachs. Evol Dev 2, 348–359 (2000).

    CAS  Article  Google Scholar 

  16. 16.

    Fukuda, K. & Yasugi, S. The molecular mechanisms of stomach development in vertebrates. DevGrowth Differ 47, 375–382 (2005).

    CAS  Article  Google Scholar 

  17. 17.

    Raghoebir, L. et al. SOX2 redirects the developmental fate of the intestinal epithelium toward a premature gastric phenotype. J Mol Cell Biol 4, 377–385, https://doi.org/10.1093/jmcb/mjs030 (2012).

    CAS  Article  PubMed  PubMed Central  Google Scholar 

  18. 18.

    Yoon, J. H. et al. Inactivation of NKX6.3 in the stomach leads to abnormal expression of CDX2 and SOX2 required for gastric-to-intestinal transdifferentiation. Mod Pathol 29, 194–208, https://doi.org/10.1038/modpathol.2015.150 (2016).

    CAS  Article  PubMed  Google Scholar 

  19. 19.

    Kim, B. M. et al. Independent functions and mechanisms for homeobox gene Barx1 in patterning mouse stomach and spleen. Development 134, 3603–3613, https://doi.org/10.1242/dev.009308 (2007).

    CAS  Article  PubMed  Google Scholar 

  20. 20.

    Ishii, Y., Rex, M., Scotting, P. J. & Yasugi, S. Region-specific expression of chicken Sox2 in the developing gut and lung epithelium: Regulation by epithelial-mesenchymal interactions. Dev Dyn 213, 464–475, https://doi.org/10.1002/(Sici)1097-0177(199812)213:4<464::Aid-Aja11>3.0.Co;2-Z (1998).

    CAS  Article  PubMed  Google Scholar 

  21. 21.

    Roberts, D. J. et al. Sonic hedgehog is an endodermal signal inducing Bmp-4 and Hox genes during induction and regionalization of the chick hindgut. Development 121, 3163–3174 (1995).

    CAS  PubMed  Google Scholar 

  22. 22.

    Shin, M., Watanuki, K. & Yasugi, S. Expression of Fgf10 and Fgf receptors during development of the embryonic chicken stomach. Gene Expr Patterns: GEP 5, 511–516, https://doi.org/10.1016/j.modgep.2004.12.004 (2005).

    CAS  Article  PubMed  Google Scholar 

  23. 23.

    Kim, B. M., Buchner, G., Miletich, I., Sharpe, P. T. & Shivdasani, R. A. The stomach mesenchymal transcription factor Barx1 specifies gastric epithelial identity through inhibition of transient Wnt signaling. Dev Cell 8, 611–622, https://doi.org/10.1016/i.devcel.2005.01.015 (2005).

    CAS  Article  PubMed  Google Scholar 

  24. 24.

    Theodosiou, N. A. & Tabin, C. J. Wnt signaling during development of the gastrointestinal tract. Dev Biol 259, 258–271 (2003).

    CAS  Article  Google Scholar 

  25. 25.

    Hryniuk, A., Grainger, S., Savory, J. G. A. & Lohnes, D. Cdx function is required for maintenance of intestinal identity in the adult. Dev Biol 363, 426–437, https://doi.org/10.1016/j.ydbio.2012.01.010 (2012).

    CAS  Article  PubMed  Google Scholar 

  26. 26.

    Brazeau, M. D. & Friedman, M. The origin and early phylogenetic history of jawed vertebrates. Nature 520, 490–497, https://doi.org/10.1038/nature14438 (2015).

    ADS  Article  PubMed  PubMed Central  Google Scholar 

  27. 27.

    Freitas, R., Zhang, G. & Cohn, M. J. Evidence that mechanisms of fin development evolved in the midline of early vertebrates. Nature 442, 1033–1037, https://doi.org/10.1038/nature04984 (2006).

    ADS  CAS  Article  PubMed  Google Scholar 

  28. 28.

    Wotton, K. R., Mazet, F. & Shimeld, S. M. Expression of FoxC, FoxF, FoxL1, and FoxQ1 genes in the dogfish Scyliorhinus canicula defines ancient and derived roles for Fox genes in vertebrate development. Dev Dyn 237, 1590–1603, https://doi.org/10.1002/dvdy.21553 (2008).

    CAS  Article  PubMed  Google Scholar 

  29. 29.

    Theodosiou, N. A. & Simeone, A. Evidence of a rudimentary colon in the elasmobranch, Leucoraja erinacea. Dev Genes Evo 222, 237–243, https://doi.org/10.1007/s00427-012-0406-8 (2012).

    CAS  Article  Google Scholar 

  30. 30.

    Montgomery, R. K., Mulberg, A. E. & Grand, R. J. Development of the human gastrointestinal tract: Twenty years of progress. Gastroenterol 116, 702–731, https://doi.org/10.1016/S0016-5085(99)70193-9 (1999).

    CAS  Article  Google Scholar 

  31. 31.

    Takei, S., Tokuhira, Y., Shimada, A., Hosokawa, M. & Fukuoka, S. Eosin-shadow method: a selective enhancement of light-microscopic visualization of pancreatic zymogen granules on hematoxylin-eosin sections. Anat Sci Int 85, 245–250, https://doi.org/10.1007/s12565-009-0067-5 (2010).

    Article  PubMed  Google Scholar 

  32. 32.

    Ishizuya-Oka, A., Hasebe, T., Shimizu, K., Suzuki, K. & Ueda, S. Shh/BMP-4 signaling pathway is essential for intestinal epithelial development during Xenopus larval-to-adult remodeling. Dev Dyn 235, 3240–3249, https://doi.org/10.1002/dvdy.20969 (2006).

    CAS  Article  PubMed  Google Scholar 

  33. 33.

    Korzh, S. et al. The interaction of epithelial Ihha and mesenchymal Fgf10 in zebrafish esophageal and swimbladder development. DevBiol 359, 262–276, https://doi.org/10.1016/j.ydbio.2011.08.024 (2011).

    CAS  Article  Google Scholar 

  34. 34.

    Sala, F. G. et al. Fibroblast growth factor 10 is required for survival and proliferation but not differentiation of intestinal epithelial progenitor cells during murine colon development. Dev Biol 299, 373–385, https://doi.org/10.1016/j.ydbio.2006.08.001 (2006).

    CAS  Article  PubMed  Google Scholar 

  35. 35.

    Tissier-Seta, J. P. et al. Barx1, a new mouse homeodomain transcription factor expressed in cranio-facial ectomesenchyme and the stomach. Mech Dev 51, 3–15 (1995).

    CAS  Article  Google Scholar 

  36. 36.

    Tendeng, C. & Houart, C. Cloning and embryonic expression of five distinct sfrp genes in the zebrafish Danio rerio. Gene Expr Patterns: GEP 6, 761–771, https://doi.org/10.1016/j.modgep.2006.01.006 (2006).

    CAS  Article  PubMed  Google Scholar 

  37. 37.

    Silberg, D. G., Swain, G. P., Suh, E. R. & Traber, P. G. Cdx1 and Cdx2 expression during intestinal development. Gastroenterol 119, 961–971, https://doi.org/10.1053/Gast.2000.18142 (2000).

    CAS  Article  Google Scholar 

  38. 38.

    Darias, M. J., Ortiz-Delgado, J. B., Sarasquete, C., Martinez-Rodriguez, G. & Yufera, M. Larval organogenesis of Pagrus pagrus L., 1758 with special attention to the digestive system development. Histol Histopathol 22, 753–768 (2007).

    CAS  PubMed  Google Scholar 

  39. 39.

    Smolka, A. J., Lacy, E. R., Luciano, L. & Reale, E. Identification of gastric H,K-ATPase in an early vertebrate, the Atlantic stingray Dasyatis-sabina. J Histochem Cytochem 42, 1323–1332 (1994).

    CAS  Article  Google Scholar 

  40. 40.

    Kageyama, T. P. progastricsins, and prochymosins: structure, function, evolution, and development. Cell Mol Life Sc 59, 288–306, https://doi.org/10.1007/S00018-002-8423-9 (2002).

    CAS  Article  Google Scholar 

  41. 41.

    Richter, C., Tanaka, T. & Yada, R. Y. Mechanism of activation of the gastric aspartic proteinases: pepsinogen, progastricsin and prochymosin. Biochem J 335(Pt 3), 481–490 (1998).

    CAS  Article  Google Scholar 

  42. 42.

    Forssell, H. Gastric mucosal defence mechanisms: a brief review. ScandJ Gastroenterol. Suppl 155, 23–28 (1988).

    Article  Google Scholar 

  43. 43.

    Godard, B. G. et al. Mechanisms of endoderm formation in a cartilaginous fish reveal ancestral and homoplastic traits in jawed vertebrates. Biol Open 3, 1098–1107, https://doi.org/10.1242/bio.20148037 (2014).

    Article  PubMed  PubMed Central  Google Scholar 

  44. 44.

    Freitas, R., Zhang, G. & Cohn, M. J. Biphasic Hoxd gene expression in shark paired fins reveals an ancient origin of the distal limb domain. PloS one 2, e754, https://doi.org/10.1371/journal.pone.0000754 (2007).

    ADS  CAS  Article  PubMed  PubMed Central  Google Scholar 

  45. 45.

    Oulion, S. et al. Evolution of repeated structures along the body axis of jawed vertebrates, insights from the Scyliorhinus canicula Hox code. Evol Dev 13, 247–259, https://doi.org/10.1111/j.1525-142X.2011.00477.x (2011).

    Article  PubMed  Google Scholar 

  46. 46.

    Theodosiou, N. A., Hall, D. A. & Jowdry, A. L. Comparison of acid mucin goblet cell distribution and Hox13 expression patterns in the developing vertebrate digestive tract. J Exp Zool B 308, 442–453, https://doi.org/10.1002/jez.b.21170 (2007).

    Article  Google Scholar 

  47. 47.

    Zeng, L. & Childs, S. J. The smooth muscle microRNA miR-145 regulates gut epithelial development via a paracrine mechanism. Dev Biol 367, 178–186, https://doi.org/10.1016/j.ydbio.2012.05.009 (2012).

    CAS  Article  PubMed  Google Scholar 

  48. 48.

    Sperber, S. M. & Dawid, I. B. barx1 is necessary for ectomesenchyme proliferation and osteochondroprogenitor condensation in the zebrafish pharyngeal arches. Dev Biol 321, 101–110, https://doi.org/10.1016/j.ydbio.2008.06.004 (2008).

    CAS  Article  PubMed  PubMed Central  Google Scholar 

  49. 49.

    Voskarides, K. ‘Plasticity-First’ Evolution and the role of miRNAs: A Comment on Levis and Pfennig. Trends Ecol Evo 31, 816–817, https://doi.org/10.1016/j.tree.2016.08.006 (2016).

    Article  Google Scholar 

  50. 50.

    Muncan, V. et al. T-cell factor 4 (Tcf7l2) maintains proliferative compartments in zebrafish intestine. EMBO reports 8, 966–973, https://doi.org/10.1038/sj.embor.7401071 (2007).

    CAS  Article  PubMed  PubMed Central  Google Scholar 

  51. 51.

    Que, J. et al. Multiple dose-dependent roles for Sox2 in the patterning and differentiation of anterior foregut endoderm. Development 134, 2521–2531, https://doi.org/10.1242/dev.003855 (2007).

    CAS  Article  PubMed  PubMed Central  Google Scholar 

  52. 52.

    Ballard, W. W., Mellinger, J. & Lechenault, H. A Series of normal stages for development of Scyliorhinus-canicula, the lesser spotted dogfish (Chondrichthyes, Scyliorhinidae). J Exp Zool 267, 318–336, https://doi.org/10.1002/Jez.1402670309 (1993).

    Article  Google Scholar 

  53. 53.

    Smolka, A. & Swiger, K. M. Site-directed antibodies as topographical probes of the gastric H,K-ATPase alpha-subunit. Biochim Biophys Acta 1108, 75–85 (1992).

    CAS  Article  Google Scholar 

  54. 54.

    Goncalves, O., Castro, L. F., Smolka, A. J., Fontainhas, A. & Wilson, J. M. The Gastric phenotype in the cypriniform loaches: A Case of reinvention? PloS one 11, e0163696 (2016).

    Article  Google Scholar 

  55. 55.

    Schmittgen, T. D. & Livak, K. J. Analyzing real-time PCR data by the comparative C(T) method. Nat Protoc 3, 1101–1108 (2008).

    CAS  Article  Google Scholar 

  56. 56.

    Freitas, R. & Cohn, M. J. Analysis of EphA4 in the lesser spotted catshark identifies a primitive gnathostome expression pattern and reveals co-option during evolution of shark-specific morphology. Dev Genes Evo 214, 466–472, https://doi.org/10.1007/s00427-004-0426-0 (2004).

    CAS  Article  Google Scholar 

  57. 57.

    Coolen, M. et al. The dogfish Scyliorhinus canicula: A reference in jawed vertebrates. CSH protocols 2008, pdbemo111, https://doi.org/10.1101/pdb.emo111 (2008).

    Article  Google Scholar 

Download references

Acknowledgements

We acknowledge Fundação para a Ciência e a Tecnologia for the support to OG (SFRH/ BD/79821/ 2011) and RF (IF/00146/2013). JMW was supported by grants from NSERC and the Canadian Foundation for Innovation. This work was funded by Coral—Sustainable Ocean Exploitation (Norte-01-0145-FEDER-000036), a project supported by the North Portugal Regional Operational Program (NORTE 2020), under the PORTUGAL 2020 Partnership Agreement, through the European Regional Development Fund (ERDF) and by the European Regional Development Fund (ERDF) through the COMPETE - Operational Competitiveness Programme and POPH - Operational Human Potential Programme and national funds through FCT–Foundation for Science and Technology (UID/Multi/04423/2013). The work was also partially funded by FEDER funds through the COMPETE 2020 Programme and National Funds through FCT - Portuguese Foundation for Science and Technology under the project number POCI-01-0145-FEDER-030562. We also would like to thank the technicians of the Facility of Aquatic Organisms at Ciimar and to A. Águas and F. Barroso, who contributed to the execution of the experiments.

Author information

Affiliations

Authors

Contributions

J.W., R.F. and L.F.C.C. designed research. O.G., R.F., G.Z., P.F., S.M., M.J.C., L.F.C.C. and J.W. performed research. O.G., R.F., P.F., M.A., G.Z., J.W. and L.F.C.C. analysed data. O.G., R.F., L.F.C.C. and J.W. wrote the manuscript with contributions from all authors.

Corresponding authors

Correspondence to Renata Freitas or L. Filipe C. Castro or Jonathan M. Wilson.

Ethics declarations

Competing Interests

The authors declare no competing interests.

Additional information

Publisher’s note: Springer Nature remains neutral with regard to jurisdictional claims in published maps and institutional affiliations.

Rights and permissions

Open Access This article is licensed under a Creative Commons Attribution 4.0 International License, which permits use, sharing, adaptation, distribution and reproduction in any medium or format, as long as you give appropriate credit to the original author(s) and the source, provide a link to the Creative Commons license, and indicate if changes were made. The images or other third party material in this article are included in the article’s Creative Commons license, unless indicated otherwise in a credit line to the material. If material is not included in the article’s Creative Commons license and your intended use is not permitted by statutory regulation or exceeds the permitted use, you will need to obtain permission directly from the copyright holder. To view a copy of this license, visit http://creativecommons.org/licenses/by/4.0/.

Reprints and Permissions

About this article

Verify currency and authenticity via CrossMark

Cite this article

Gonçalves, O., Freitas, R., Ferreira, P. et al. Molecular ontogeny of the stomach in the catshark Scyliorhinus canicula. Sci Rep 9, 586 (2019). https://doi.org/10.1038/s41598-018-36413-0

Download citation

Further reading

Comments

By submitting a comment you agree to abide by our Terms and Community Guidelines. If you find something abusive or that does not comply with our terms or guidelines please flag it as inappropriate.

Search

Quick links

Nature Briefing

Sign up for the Nature Briefing newsletter — what matters in science, free to your inbox daily.

Get the most important science stories of the day, free in your inbox. Sign up for Nature Briefing