Skeletal myogenesis serves as a paradigm to investigate the molecular mechanisms underlying exquisitely regulated cell fate decisions in developing embryos. The evolutionarily conserved miR-133 family of microRNAs is expressed in the myogenic lineage, but how it acts remains incompletely understood. Here, we performed genome-wide differential transcriptomics of miR-133 knockdown (KD) embryonic somites, the source of vertebrate skeletal muscle. These analyses, performed in chick embryos, revealed extensive downregulation of Sonic hedgehog (Shh) pathway components: patched receptors, Hedgehog interacting protein and the transcriptional activator Gli1. By contrast, Gli3, a transcriptional repressor, was de-repressed and confirmed as a direct miR-133 target. Phenotypically, miR-133 KD impaired myotome formation and growth by disrupting proliferation, extracellular matrix deposition and epithelialization. Together, these observations suggest that miR-133-mediated Gli3 silencing is crucial for embryonic myogenesis. Consistent with this idea, we found that activation of Shh signalling by either purmorphamine, or KD of Gli3 by antisense morpholino, rescued the miR-133 KD phenotype. Thus, we identify a novel Shh/myogenic regulatory factor/miR-133/Gli3 axis that connects epithelial morphogenesis with myogenic fate specification.
Skeletal muscle is important for mobility and survival. Its development is a highly regulated process, involving developmental signals and their effector pathways, a hierarchy of transcription factors – the myogenic regulatory factors (MRFs), and post-transcriptional regulation by noncoding RNAs (Buckingham and Rigby, 2014; Mok and Sweetman, 2011).
In vertebrate embryos, skeletal muscles of the trunk and limbs are derived from somites, transient paired segments that form in a regular sequence on either side of the neural tube and notochord (Christ and Scaal, 2008). In response to signals, including Wnt, Shh and Notch (Abou-Elhamd et al., 2015; Abu-Elmagd et al., 2010; Borycki et al., 1999; Johnson et al., 1994; Münsterberg et al., 1995; Rios et al., 2011; Sieiro et al., 2016), the initially epithelial somite undergoes morphogenetic changes and differentiates. On the ventral side, cells dissociate to form the sclerotome, whilst the dermomyotome on the dorsal side remains epithelial and contributes myocyte progenitors to the myotome. Myotome formation initiates at the epaxial lip of the dermomyotome, abutting the neural tube (Gros et al., 2004). Interactions with migrating neural crest cells triggers translocation of dermomyotomal lip progenitors into the myotome, where they orientate, elongate and begin to differentiate into myocytes (Rios et al., 2011; Sieiro et al., 2016).
Shh, derived from the notochord and floor plate, activates myogenesis (Münsterberg et al., 1995), and is essential for the activation of the myogenic determination gene, Myf5, in epaxial muscle progenitor cells in mice (Borycki et al., 1999; Gustafsson et al., 2002), or in both epaxial and hypaxial domains in avian embryos (Kahane et al., 2013). Myf5 activation is mediated via Gli activator proteins, Gli1 and Gli2, acting on a Gli-binding site in the mouse epaxial enhancer (Gustafsson et al., 2002; McDermott et al., 2005; Teboul et al., 2002). In the absence of Shh, the Gli3 repressor inhibits Myf5 transcription (McDermott et al., 2005). Furthermore, in both avian and mouse embryos, Shh signalling is crucial for the transition from proliferating Pax7-positive progenitors to terminally differentiating myocytes (Kahane et al., 2013).
MicroRNAs (miRNAs or miRs) are short noncoding RNAs that bind to target sites located in 3′UTRs of mRNAs. This interaction leads to inhibition of translation, mRNA cleavage and transcript degradation via deadenylation (Bartel, 2009; Béthune et al., 2012). Through their effects on target gene expression, miRNAs regulate developmental timing and provide robustness to cell fate decisions (Ebert and Sharp, 2012; Hornstein and Shomron, 2006). The miR-1, miR-206 and miR-133 families, comprising miR-1-1/2, miR-206 and miR-133a/b, are encoded by three loci in mouse and human, and by four loci in chicken (Sweetman et al., 2008). One member of each family is produced from the same primary transcripts and they play important roles in regulating proliferation, differentiation and cell fate specification in developing muscle (Horak et al., 2016; Mok et al., 2017). In mouse and chicken embryos, miR-1/miR-133a are expressed in skeletal and cardiac muscle. By contrast, miR-206/miR-133b are expressed in myoblasts of somites, limb buds and head muscles, but not in cardiomyocytes (Darnell et al., 2006; Sweetman et al., 2008). In Xenopus and zebrafish, the miR-1, miR-206 and miR-133 families are present in skeletal muscle but are not detected in the heart (Ahmed et al., 2015; Mishima et al., 2009). Together with myocyte enhancer factor-2 (MEF2) proteins, the MRFs regulate expression of miR-1, miR-206 and miR-133 in somites (Liu et al., 2007; Sweetman et al., 2008) and in C2C12 myoblasts (Rao et al., 2006; Rosenberg et al., 2006). In C2C12 myoblasts, the miR-1, miR-206 and miR-133 families regulate the balance between differentiation and proliferation through interactions with multiple targets (Alteri et al., 2013; Chen et al., 2006; Feng et al., 2013; Goljanek-Whysall et al., 2012).
We previously used miRNA knockdown (KD) in chick somites to show that miR-1, miR-206 and miR-133 negatively regulate BRG1/BRM-associated factor 60 (BAF60) variants BAF60A and BAF60B. This facilitates the preferential incorporation of BAF60C into the BAF protein/BRG1 chromatin remodelling complex required for myogenesis (Goljanek-Whysall et al., 2014). In earlier somites, miR-206 facilitates the complete downregulation of Pax3 in the myotome, ensuring timely transition of myogenic progenitor to committed myoblast (Goljanek-Whysall et al., 2011). Studies in mice showed that miR-133a isoforms are essential for the maintenance of skeletal muscle structure and myofibre identity (Liu et al., 2011), and for controlling brown fat differentiation through targeting Prdm16 (Trajkovski et al., 2012); although deletion of the miR-206/133b cluster did not result in skeletal muscle defects (Boettger et al., 2014). In zebrafish, transcriptomic analysis revealed the importance of miR-1 and miR-133 for sarcomeric actin organization (Mishima et al., 2009). However, the functions of miR-133 in early myogenesis remain unclear.
Here, we characterize the mechanisms that underlie the embryonic phenotype resulting from antagomir-mediated miR-133 KD in avian somites. Impaired myogenesis was evident from reduced expression of MRFs, reduced cell proliferation and impaired growth of the dermomyotome and myotome, as well as reduced actin accumulation and disorganized basement membrane (BM) deposition. Differential transcriptomics of miR-133 KD somites identified negative effects on Shh pathway components, suggesting a role for miR-133 in modulating Shh signalling. Expression of the Gli3 transcriptional repressor was de-repressed after miR-133 KD, and luciferase assays confirmed direct regulation via a functional target site in the Gli3 3′UTR that is complementary to the miR-133 seed sequence. Myotome formation and epithelialization, BM deposition and myogenic differentiation were restored in miR-133 KD somites by concomitant activation of Shh signalling using purmorphamine, a synthetic agonist of the smoothened (Smo) receptor (Sinha and Chen, 2006), or by the concomitant morpholino (MO)-mediated knockdown of Gli3 repressor. Our data identify a novel Shh/MRF/miR-133/Gli3 axis and show that stabilization of myogenic differentiation and growth of the myotome require the negative regulation of Gli3 by miR-133.
miR-133 is expressed in nascent myoblasts
The spatiotemporal expression of miR-133 was determined by whole-mount in situ hybridization. In Hamburger Hamilton (HH) stage 15 chick embryos (Hamburger and Hamilton, 1951), miR-133 was detected in early stage somites (sIII/IV) and in differentiating somites. Expression was also seen in the neural tube, brain, anterior notochord, mesonephric duct and heart (Fig. S1A). In early somites, which begin to de-epithelialize ventrally, expression was detected adjacent to the neural tube, where the first myoblasts emerge. The relative expression levels of miR-133 increased as somites matured, and in differentiating somites miR-133 was restricted to the myotome (Fig. S1A,B), as previously reported for older-stage embryos (Goljanek-Whysall et al., 2011; Sweetman et al., 2008).
miR-133 coordinates cell fate acquisition with somite morphogenesis
Somites are severely affected by antagomir-mediated KD of miR-133, with epithelial morphology lost in the dermomyotome and myotome, and myogenin (Mgn) expression either lost completely (80%) or partially (20%), indicating that by 24 h, myogenesis is compromised (Figs 1B and 4B) (Goljanek-Whysall et al., 2014).
To characterize in more detail the underlying cellular and molecular mechanisms, we established that effects resulting from miR-133 inhibition were first detected after 9 h. Epithelial somites of HH14/15 embryos injected with fluorescein isothiocyanate (FITC)-labelled antagomir-133 (AM133) and examined after 6, 9, 12 or 24 h (Fig. 1A) showed partial loss of Myf5, MyoD (Fig. S2A) and Mgn expression 9 h after miR-133 KD (Fig. 1B). No phenotype was detected after 6 h, and after 12 and 24 h, phenotypes were more pronounced (Fig. 1B, Fig. S2B). Control injections of scrambled antagomir (AMscr) had no effect (Fig. S3A-D). Reverse transcription quantitative polymerase chain reaction (RT-qPCR) confirmed significantly reduced abundance of miR-133 in somites after AM133 injection (Fig. 1C), also observed with northern blot analysis (Goljanek-Whysall et al., 2014). Interestingly, AM133 injections of the equivalent, interlimb-level somites at later stages (HH20), when miR-133 is expressed in a more developed myotome, did not lead to myogenic defects (Fig. S2C), suggesting a critical window in younger, less mature somites, in which miR-133 function is essential.
Pax3 and Pax7 immunostaining of cryosections revealed a reduced dermomyotome size, confirmed by pixel measurements using Fiji/ImageJ, in AM133-injected somites compared with somites from the contralateral noninjected side (HH14/15) (Fig. 2A,B). Phosphor histone H3 (pH3) staining showed fewer mitotic cells present in the dermomyotome and myotome, indicating impaired cell proliferation after miR-133 KD (Fig. 2C). Immunostaining for caspase-3 (Cas3) showed no detectable increase in apoptotic cells (Fig. S2D). AMscr injections did not affect dermomyotome proliferation or size (Fig. S3A-C).
Epithelial organization of the dermomyotome, assessed by actin staining, showed a reduced number of apicobasal-orientated dermomyotomal cells. Furthermore, the dermomyotomal lip was poorly defined, had lost its epithelial character and had less actin accumulated than in the same structure in noninjected somites (Fig. 2D). In addition, discontinuous and disorganized laminin staining suggested that BM deposition was impaired, and a BM had not fully formed on the basal side of dermomyotome cells or beneath the myotome (Fig. 2D). The BM surrounding the neural tube remained unaffected, and AMscr injections did not affect epithelial organization of the dermomyotome (Fig. S3D).
Inhibition of miR-133 affects Shh pathway components
The discrete molecular and cellular changes observed after 9 h in the dermomyotome and myotome following AM133 injection culminate in severe impairment of myogenesis by 24 h (Figs 1 and 2, Figs S2 and S3). Genome-wide differential transcriptomics of AM133- or AMscr-injected somites was used to identify the pathways and cellular processes involved (Fig. 3, Fig. S4). This was performed at 9 h to capture the earliest events. Hierarchical clustering confirmed that AM133-injected somites were more similar to each other than to control somites, and identified differentially expressed (DE) genes (Fig. 3B). Gene ontology (GO) analysis showed that the genes involved in processes relating to cell division were significantly decreased (Fig. 3C), consistent with observations that dermomyotome size and number of mitotic cells were reduced after miR-133 KD.
Amongst the top 50 significantly downregulated DE genes were myogenic markers, Myf5 and MyoD, and sclerotome markers, Pax1 and Pax9. Strikingly, several Shh pathway components were also in this group, including patched-1 (Ptch1) and patched-2 (Ptch2) receptors, Hedgehog interacting protein (Hhip) and the transcriptional activator Gli1 (Fig. 3B,D). Thus, we looked for a transcriptional repressor of Shh pathway genes amongst the genes for which relative expression was increased. A strong candidate was Gli3, which was amongst the top 200 de-repressed genes and its expression was significantly increased (P=0.03) (Fig. 3D). Gli3 was therefore a putative direct target gene for miR-133. A miR-133 target site identified in its 3′UTR – conserved in human, chimp, mouse, cow and frog – was validated by luciferase reporter assays. Reporter gene expression was inhibited significantly after transfection of miR-133. Introducing mutations into the 8-mer seed sequence of the target site restored reporter gene expression even in the presence of miR-133 (Fig. 3E), confirming its importance. A control miRNA had no effect. Furthermore, analysis of Gli3 protein levels by western blotting confirmed a relative increase of the short repressor isoform (Gli3Rep) in somites following miR-133 inhibition in vivo using AM133 injection compared with control AMscr-injected somites (Fig. 3F).
Shh pathway activation rescues miR-133 KD
The finding that Gli3, which acts predominantly as a transcriptional repressor, is a direct target for miR-133 and de-repressed after miR-133 KD (Fig. 3D,F), led us to test whether pharmacological activation of the Shh pathway can rescue the myogenic phenotype. Knockdown of miR-133 completely inhibited myogenesis after 24 h (Figs 1B and 4B, Fig. S2B). However, co-injection of AM133 and purmorphamine, an activator of Shh signalling (Fig. 4A), restored myogenic differentiation, as shown by expression of Mgn (Fig. 4B). To determine whether Gli3 de-repression was crucial for the phenotype observed, we knocked down Gli3 expression using MOs and examined whether this could rescue the AM133-induced loss of Mgn. A FITC-labelled Gli3-translation-blocking MO was electroporated concomitant with AM133 injection (Fig. 4C,D). Western blots of transfected somites showed that Gli3Rep protein was reduced by Gli3 MO compared with control MO (Fig. S3F). A faint band representing the full-length Gli3 activator (Gli3Act) was present in both samples, consistent with the finding that Gli3Act becomes rapidly degraded (Wen et al., 2010). In situ hybridization showed that Gli3 MO restored myogenesis in AM133-treated somites (Fig. 4D), suggesting that miR-133 mediates its effects via negative regulation of Gli3.
Somite organization was improved after treatment with purmorphamine or the concomitant transfection of Gli3 MO together with AM133; however, the somites were smaller (Fig. 4B,D). Thus, we examined the rescue phenotype in more detail, after 9 h when Mgn expression appeared normal (Fig. S5). Pax3 and Pax7 immunostaining showed that although the dermomyotome was smaller, its epithelial nature was preserved in somites injected with AM133 and purmorphamine (Fig. 5A-D). Fewer mitotic cells were detected by pH3 staining, compared with contralateral somites (Fig. 5C), and this was similar to observations in somites injected with AM133 alone (Fig. 2C). Actin and laminin staining showed that epithelial character and BM deposition were restored around the dermomyotome and myotome (Fig. 5D).
Finally, AM133 co-injection with purmorphamine restored expression levels of DE hedgehog pathway genes (Fig. 6A). Somites injected with AMscr, or with AM133 alone, or with AM133 and purmorphamine, were examined using RT-qPCR. Expression of Gli1, Gli2, Ptch1, Smo and Hhip was decreased in somites injected with AM133, whereas expression of Gli3 increased, consistent with the differential transcriptomics data. Purmorphamine co-injection with AM133 led to recovery of Shh pathway components compared with somites injected with AM133 alone. The exception was Gli3 expression, which remained de-repressed. This was not unexpected given that miR-133 function was still inhibited by antagomir-133 (Fig. 6A). The relative expression of Pax3 and Pax7 increased, whilst that of Myf5 and Mgn decreased, after antagomir-133 injection. Myf5 was also significantly decreased after miR-133 KD in the differential transcriptomics data (Fig. 3B). Co-injection of purmorphamine with AM133 restored expression of pre-myogenic markers, Pax3 and Pax7, to levels comparable to those of control somites, and Myf5 and Mgn levels were also rescued (Fig. 6B). In addition, expression of Snail1, a gene associated with epithelial mesenchymal transition (EMT), or gremlin 1 (Grem1), a BMP antagonist was rescued by Shh pathway activation (Fig. 6D). However, interestingly, genes associated with proliferation, Cdc20, Cdk1 and Fgf8, remained repressed, consistent with fewer pH3-positive cells and smaller somites in the presence of AM133, irrespective of the presence of purmorphamine. This suggests that myogenic differentiation and epithelialization are uncoupled from proliferation and that there is differential sensitivity of these processes for GliAct/GliRep balance. Furthermore, there might be additional functions of miR-133, independent of Gli3 targeting and Shh pathway regulation.
Despite recent progress, we still do not have a complete understanding of how myogenic progenitor cells, once specified, can stably execute their differentiation programme. miRNAs are involved in the fine tuning of developmental processes, and we use the accessibility of chicken embryos to investigate the function of the miR-133 family in vivo, during embryonic myogenesis using antagomir-mediated inhibition, differential transcriptomics and rescue experiments.
Embryonic loss of function of miRNAs is often difficult to investigate owing to functional redundancy of almost identical mature miRNAs produced from multiple genetic loci, thus making reverse genetic approaches in mice challenging. Observations from mice with genetic deletion of miR-133a-1 and miR-133a-2 family members suggest a role for adult skeletal muscle homeostasis (Liu et al., 2011). By contrast, removal of the miR-206/133b cluster did not reveal essential functions in skeletal muscle differentiation or regeneration (Boettger et al., 2014). The concomitant knockout (KO) of the miR-1-1/133a-2 and miR-1-2/133a-1 clusters, which are expressed in cardiac and skeletal muscle, led to an early cardiac defect (Wystub et al., 2013). However, an embryonic skeletal muscle phenotype was not reported in any of these lines, most likely due to expression from unaffected loci. Chick embryos offer the opportunity to perform conditional miRNA KD experiments using antagomirs that simultaneously inhibit the mature form of all miR-133 family members produced (Goljanek-Whysall et al., 2014). This has uncovered a crucial function of miR-133 in the modulation of Shh signalling through direct targeting of Gli3, a transcriptional repressor of the pathway and of myogenesis (McDermott et al., 2005; Wen et al., 2010).
Shh signals, derived from the notochord and floorplate, activate myogenesis in explants of presegmented mesoderm and act on myogenic progenitors in the dermomyotome and dermomyotome lip (Borycki et al., 1999, 1998; Münsterberg et al., 1995). This induces expression of Myf5 via Gli activator proteins. Myf5 activates expression of miR-133 via upstream E-boxes (Rao et al., 2006; Rosenberg et al., 2006; Sweetman et al., 2008), and we show here that miR-133 directly targets Gli3 via a conserved site in the 3′UTR (Fig. 3E). This site is conserved and was shown to be functional in human Sertoli cells (Yao et al., 2016). We suggest a model in which Gli3 silencing by miR-133 maintains the finely tuned balance of Gli activator and repressor forms during myogenesis (Fig. 3F). Thus, post-transcriptional silencing of Gli3 in nascent myoblasts promotes the stable activation of the skeletal muscle differentiation programme in response to the Gli activators Gli1 and Gli2 (Fig. 6E). This model is consistent with the finding that concomitant Gli3 knockdown using a MO restored myogenic differentiation after miR-133 KD (Fig. 4D). In addition, miR-133 expression, which is initiated by Myf5 in early myoblasts, is mutually exclusive with Gli3 (Fig. S1) (Berti et al., 2015; Mok et al., 2015; Sweetman et al., 2008). In early somites, Gli3 transcripts are excluded from Myf5/miR-133-expressing myoblasts and restricted to the dermomyotome, including the dermomyotome lip (Fig. S1C). In differentiating somites, in which the myogenic programme is stably established, miR-133 and Gli3 remain expressed in a mutually exclusive fashion, in the myotome or dermomyotome, respectively (Goljanek-Whysall et al., 2014; Kahane et al., 2013). In later-stage somites, AM133 injection had no effect on myogenin expression (Fig. S2C), suggesting that miR-133 function is essential specifically during early myogenesis. In addition, the lack of a detectable phenotype at later stages shows that there are no nonspecific, off-target or toxic effects.
De-repression of Gli3 transcript and protein following miR-133 KD led to inhibition of the Shh pathway (Figs 3B,D,F and 6A), including the downregulation of Gli1 activator, which is important for Myf5 activation (Gustafsson et al., 2002; McDermott et al., 2005). Our results imply direct and indirect consequences resulting from disruption of the Gli1/2 and Gli3 balance in early somites. It is likely that early myoblasts are directly affected, with miR-133 KD leading to loss of stable myogenesis, after initial expression of MRFs (Fig. 1B). The finding that concomitant Gli3 KD, using electroporation of a Gli3 MO (Fig. 4D, Fig. S3F), rescued myogenic gene expression suggests that miR-133 mediated post-transcriptional regulation of Gli3 is crucial to stably establish the myogenic programme. However, myogenic differentiation also involves extracellular matrix production and thus dermomyotome epithelial organization could be affected indirectly.
Shh signal response genes expressed in the myotome include Ptch1 and Ptch2 (Pearse et al., 2001), Gli1, Hhip (Kahane et al., 2013), which attenuates signalling (Chuang and McMahon, 1999; Ingham and McMahon, 2001), Fgf8 (Smith et al., 2005) and the myogenic determination gene, Myf5 (Borycki et al., 1998; McDermott et al., 2005). Differential transcriptomics and RT-qPCR data showed that these genes are negatively affected by miR-133 KD in developing somites (Figs 3B,D and 6A-C). Thus, they are secondary targets of miR-133, but might be directly regulated by Gli3 repressor (Fig. 3F). Using motif searches we found potential Gli binding sites within 2 kb upstream of transcription start sites in chicken Ptch1, Ptch2, Myf5 and Fgf8 genes, consistent with Ptch1 and Myf5 being direct targets for Gli proteins (Cohen et al., 2015; Gustafsson et al., 2002).
Other genes downregulated after miR-133 inhibition, such as cell cycle associated genes, Cdk1 and Cdc20, or sclerotome genes, Pax1 and Pax9 (Fig. 3B), are likely to be indirectly affected through feedback mechanisms and/or noncell-autonomous mechanisms. For example, the significant downregulation of Fgf8 could explain effects on cell proliferation and growth as well as on sclerotome differentiation (Figs 3B and 6C). In addition, BMP signals cooperate with Shh to activate somitic chondrogenesis (Murtaugh et al., 1999; Zeng et al., 2002). BMP signalling is likely to be inhibited after miR-133 KD, because Grem1, a BMP antagonist, is amongst the top 50 de-repressed genes (Fig. 3B). This provides a possible explanation for negative effects on Pax1 and Pax9 expression. Interestingly, in developing limb buds, Gli3 specifies digit identities by promoting cell cycle exit and BMP-dependent chondrogenic differentiation via controlling Grem1 expression (Lopez-Rios et al., 2012).
The role of Gli2 is less clear at present. Although we cannot exclude that Gli2 also contributes to the negative regulation of Shh pathway components, we think that this is less likely. Differential transcriptomics showed that Gli2 was slightly de-repressed; however, this change was not significant (Fig. 3D) and was not confirmed by RT-qPCR (Fig. 6A), and the Gli2 3′UTR has no predicted miR-133 target site. Expression patterns of Gli transcription factors in chick somites are more consistent with the idea that Gli3 is the main repressor of the myogenic programme: Gli1 and Gli2 are expressed in both dermomyotome and myotome; however, Gli3 is excluded from the myotome (Borycki et al., 1998; Kahane et al., 2013).
The effect of miR-133 KD on somite differentiation is dramatic. Expression of myogenic differentiation genes and epithelial organization of the dermomyotome and myotome are severely affected (Figs 1 and 2, Fig. S2A,B). It has been shown that Shh is important for laminin alpha 1 synthesis in the myotome (Anderson et al., 2009), thus suggesting miR-133 KD, and the resulting Gli3 de-repression might lead to disrupted BM assembly, owing to effects on laminin activation. Co-injection with purmorphamine restored BM deposition, indicating that rescue of Gli1, and to some extent Gli2, expression restores the balance of Gli proteins sufficiently to allow laminin synthesis, even in the presence of elevated Gli3 levels (Figs 4E and 5D).
Shh is also required to maintain the epithelial character of the dermomyotome (Kahane et al., 2013), which was disrupted upon miR-133 KD (Fig. 2C) and rescued by purmorphamine co-injection with AM133 (Fig. 5D). Purmorphamine-mediated rescue confirms that stabilization of the myogenic differentiation programme is intimately linked with cellular organization, and both depend on Shh pathway activity (Fig. 6E). This is in line with the close integration of epithelial morphology and cell fate determination mediated by Notch, GSK3β and Snail1 during the initiation of myogenesis (Sieiro et al., 2016). On the other hand, myogenesis and epithelialization were uncoupled from proliferation. Proliferation was not rescued owing to the continued de-repression of Gli3, which might affect expression of mitotic signals, such as Fgf8, and cell cycle regulators, Cdc20 and Cdk1 (Fig. 6A,C). Similar observations have previously been made in the limb (Lopez-Rios et al., 2012) and the neural tube (Cayuso et al., 2006; Ulloa et al., 2007). Finally, it has been reported that Shh causes premature myogenic differentiation (Borycki et al., 1999; Kahane et al., 2001, 2013), which could also explain why proliferation was not rescued.
Together, our data uncover a novel Shh/MRF/miR-133/Gli3 axis by which miR-133 and its modulation of the Shh signalling pathway via the direct targeting of Gli3 enable the coordination of epithelial morphology with stabilization of the cellular differentiation programme during early myogenesis.
MATERIALS AND METHODS
Fertilized eggs (Henry Stewart) were incubated until the desired stage of development (Hamburger and Hamilton, 1951). Antagomir-133 (AM133) and a scrambled sequence (AMscr), with final concentration of 1 µM, were designed as previously described (Goljanek-Whysall et al., 2011). The posterior six somites of HH14/15 embryos, or the equivalent interlimb-level somites of HH20 embryos, were injected. Embryos were harvested and processed for in situ hybridization or immunohistochemistry, or injected somites were dissected and processed for RNA or protein extraction. Purmorphamine (Sigma-Aldrich) was dissolved in dimethyl sulfoxide (DMSO) (2 μM) (Dessaud et al., 2007) and co-injected with antagomir. Gli3 antisense MO was 3′ FITC-labelled (Gene Tools) (Table S1). Gli3 MO was co-injected with AM133 into the posterior six somites of HH14/15 embryos, followed by electroporation using six 10-ms pulses of 60 V.
In situ hybridization, immunohistochemistry and image analysis
Whole-mount in situ hybridization using digoxigenin-labelled LNA oligo probe for miR-133a (Exiqon) or antisense RNA probes for Pax3, Myf5, MyoD, Mgn, Gli3 (a gift from Matt Towers, University of Sheffield, Sheffield, UK) was carried out as described previously (Goljanek-Whysall et al., 2011). Antagomirs were detected using anti-FITC antibody coupled to alkaline phosphatase (Roche) as previously described (Goljanek-Whysall et al., 2011). Cryosections (15 μm) of 4% paraformaldehyde-fixed OCT embedded embryos were immunostained. Primary antibodies used were anti-Pax3 (1:200), anti-Pax7 (1:200), anti-laminin (1:100), from the Developmental Studies Hybridoma Bank, and anti-rabbit pH3 (1 mg/ml, Merck). Phalloidin (Invitrogen) was used at 1:100 to stain actin. Secondary antibodies were Alexa Fluor 647-conjugated anti-rabbit or anti-mouse (Invitrogen), used at 1 mg/ml in 5% bovine serum albumin/5% goat serum/PBS. DAPI (Sigma-Aldrich) was used at 0.1 mg/ml in PBS. Sections were visualized on an Axioscope with Axiovision software (Zeiss). Images were imported into Fiji/ImageJ, and areas of staining were calculated from binary images by calculating pixel numbers from injected and noninjected sides, when appropriate neural tube staining was removed. A minimum of 10 sections from three embryos were analysed for each experiment. Statistical analysis used GraphPad Prism (version 6) software. Mann–Whitney nonparametric two-tail testing was applied to determine P-values.
RNA extraction and RT-qPCR
RNA and miRNA isolation from somites was performed using RNeasy (Qiagen) and miRCURY RNA kits (Exiqon) according to the manufacturer's protocols. cDNA was synthesized from 600 ng RNA using a Maxima First Strand cDNA synthesis kit (Thermo Fisher Scientific). For miRNAs, cDNA was synthesized from 10 ng using Universal cDNA synthesis kit II (Exiqon). RT-qPCR was performed on a 7500 Fast Real Time PCR machine (Applied Biosystems) using SYBR Green PCR Master Mix (Thermo Fisher Scientific) according to the manufacturer's instructions. Primers for the miR-133a sequence 5′-UUGGUCCCCUUCAACCAGCUGU-3′, were designed by Exiqon. Other primers (Sigma-Aldrich) (Table S1) were designed with Primer3 software (http://biotools.umassmed.edu/bioapps/primer3_www.cgi). RT-qPCR was normalized to Gapdh for mRNA, or Rnu6 for miRNA, based on Exiqon protocols. Three independent experiments each with three replicate samples were performed for each RT-qPCR. The ΔΔCT (Livak and Schmittgen, 2001) method was used to analyse gene expression levels. Statistical analysis was performed as previously described.
Sequencing libraries were built according to Illumina Standard Protocols (Earlham Institute). Each sample contained pooled, injected somites from ten embryos. Sequencing was performed on one lane of a flow cell on an Illumina HiSeq2500 platform. cDNA was end-paired, A-tailed and adapter-ligated before amplification and size selection. Library QC used a gel and a bioanalyser. Transcript abundances for each sample were estimated with Kallisto (Bray et al., 2016) using the Gallus gallus reference cDNA set (Galgal5) downloaded from Ensembl (Yates et al., 2016). Differential expression between antagomir-133 (AM133)- and scrambled (AMscr)-injected samples was calculated using DESeq (Anders and Huber, 2010), with an adjusted P-value significance threshold of 0.05. The data have been uploaded to the NCBI SRA, under accession number PRJNA384007. GO term analysis was performed using the DAVID Bioinformatics Resources 6.8, available at https://david.ncifcrf.gov/. Statistical analysis was performed using false discovery rate (FDR).
DNA constructs, transfections and luciferase assay
Sensor constructs contained a chick Gli3 3′UTR fragment in a modified pGL3 vector (Promega); for primers see Table S1. Mutant construct replaced the miR-133a seed site GGGACCA with the sequence GTTGACAA. Chick dermal fibroblast (DF1) cells were transfected in 96-well plates with 200 ng luciferase reporter plasmid with miR-133 or control (50 nM, Sigma-Aldrich) using Lipofectamine 2000 (Invitrogen). A Renilla luciferase plasmid was included to normalize for transfection efficiency and transfections used triplicate samples. The miRNA mimics were identical to mature miRNA; sequences are listed in Table S1. Firefly and Renilla luciferase activity was measured after 24 h using a multilabel counter (Promega GloMax), and relative activity was calculated for each sample.
Primary cell culture and western blotting
Somites of wild-type embryos were dissected and cultured in Dulbecco's modified Eagle medium, 10% fetal bovine serum, 1% penicillin/streptomycin for 4 h before being transfected with Gli3 MO (1 mM) or control MO (1 mM) using Endoporter PEG (Gene Tools) and protein extracted after 48 h. Somites from AM133- or AMscr-injected embryos were dissected for protein extraction. Protein lysate (31.5 μg) was run on pre-cast 4-15% polyacrylamide gels (Bio-Rad) and blotted onto polyvinylidene fluoride membrane (Bio-Rad). Primary antibody against Gli3 (1:200, 6F5 Gli3N, Genentech, Wen et al., 2010) was applied at 4°C overnight before secondary polyclonal goat anti-mouse HRP (1:1000, P0447, DAKO) was applied for 1 h at room temperature. The blots were treated with an ECL substrate kit (GE Healthcare) and imaged. Primary antibody against actin (1:1000, ab3280, Abcam) was applied at 4°C overnight; secondary polyclonal goat anti-mouse HRP was applied for 1 h at room temperature. The blots were treated with an ECL substrate kit and imaged. Quantification of blots was performed using ImageJ.
We thank all members of the Münsterberg and Wheeler laboratories for discussions, James Briscoe and Matt Towers for sharing plasmids, and Paul Thomas for assistance with microscopy.
Conceptualization: G.F.M., G.W., A.M.; Methodology: A.M.; Validation: G.F.M., E.L.-V., E.M., C.V.; Formal analysis: S.M.; Investigation: G.F.M., E.L.-V., E.M., C.V.; Data curation: S.M.; Writing - original draft: A.M.; Writing - review & editing: G.F.M., G.W., A.M.; Visualization: G.F.M., E.L.-V., E.M., C.V., S.M.; Supervision: A.M.; Project administration: A.M.; Funding acquisition: A.M.
This work was supported by the Biotechnology and Biological Sciences Research Council (BB/K003437 and BB/N007034 to A.M.). E.L.-V. was funded by an H2020 Marie Skłodowska-Curie Actions Individual Fellowship (705089). Deposited in PMC for immediate release.
RNA sequencing data are available at the NCBI SRA, under accession number PRJNA384007.
The authors declare no competing or financial interests.