Abstract
During development cell commitment is regulated by inductive signals that are tightly controlled in time and space. In response, cells activate specific programmes, but the transcriptional circuits that maintain cell identity in a changing signalling environment are often poorly understood. Specification of inner ear progenitors is initiated by FGF signalling. Here, we establish the genetic hierarchy downstream of FGF by systematic analysis of many ear factors combined with a network inference approach. We show that FGF rapidly activates a small circuit of transcription factors forming positive feedback loops to stabilise otic progenitor identity. Our predictive network suggests that subsequently, transcriptional repressors ensure the transition of progenitors to mature otic cells, while simultaneously repressing alternative fates. Thus, we reveal the regulatory logic that initiates ear formation and highlight the hierarchical organisation of the otic gene network.
Similar content being viewed by others
Introduction
Unravelling the structure of regulatory circuits that control development provides mechanistic insight into the assembly of a body plan and functional organs. Experimental perturbation combined with network inference offers a powerful approach to establish the topology of regulatory networks and to predict the mechanisms underlying biological processes. Here we use the vertebrate inner ear as a model to study how signalling events initiate a developmental programme and how this programme is subsequently stabilized. The inner ear arises from a simple epithelium, the otic placode, which in amniotes is first visible at the 10 somite stage (ss) as a sheet of columnar cells next to rhombomeres 5 and 6 of the hindbrain1, 2. The placode then invaginates forming the otic cup, which separates from the surface ectoderm to generate the otic vesicle. The vesicle gradually acquires the architecture of the adult inner ear through morphogenetic changes accompanied by the differentiation of a large number of specialised cell types.
At placode stages, cells are committed to inner ear fate, but prior to this, are part of a progenitor pool with the potential to contribute to other sense organs and to cranial sensory ganglia. These precursors are confined to a band of ectoderm that surrounds the anterior neural plate, which has been termed the pre-placodal region (PPR)3,4,5,6,7. Under the influence of fibroblast growth factor (FGF) signalling progenitor potential is restricted and cells become specified as otic-epibranchial precursors (OEPs)8,9,10,11,12,13,14,15,16,17,18,19. Initially FGFs emanate from the underlying mesoderm like FGF19 in chick and FGF10 in mouse, while later hindbrain derived FGF3 contributes to OEP induction9, 18. It has been suggested that thereafter reduction of FGF signalling maybe required20 before a combination of Wnt and Notch signalling promotes otic identity20,21,22. Thus, complex signalling events gradually commit sensory progenitors to the otic lineage.
Downstream of these signals a number of transcription factors are activated, which in turn are required for otic specification1. However, only a few factors respond to FGF signalling8, 14, 17, 23, and among these many become expressed only at later stages (e.g. Foxg1, Sox10), after otic cells are specified and maintain their character in the absence of additional signalling24, 25. These findings suggest that a small regulatory network may act immediately downstream of FGF to stabilise OEP identity prior to otic commitment. To explore this, we took advantage of an established in vitro system to modulate FGF signalling over time, quantified changes of more than 100 genes expressed in otic and other placodal cells and then used a Random Forests technique to infer a gene regulatory network that models FGF action. This systems approach identifies a circuit of positive feedback loops that stabilises OEP identity in response to FGF, followed by reciprocal inhibitory interactions to refine time and space of otic gene expression and to repress alternative fates.
Results
Sensory progenitors transiently activate OEP genes in the absence of FGF signalling
At head fold stages, all placode progenitors are specified as lens, irrespective of their later fate: when cultured in isolation they initiate the lens programme and the induction of other placodes requires its repression by local inducing signals26, 27. The first step in otic induction is the formation of otic-epibranchial progenitors (OEPs) in the posterior pre-placodal region (pPPR) mediated by FGF signalling1, 28, 29. Here we explore the temporal dynamics in response to FGF during OEP induction using a well-characterised in vitro assay25.
To establish a baseline we first characterised dynamic changes of gene expression in posterior PPR explants in the absence of FGF. Posterior PPR from head fold stages (HH6) was cultured in isolation for 6, 12 or 24 hours (Fig. 1a–e). Gene expression in 7–10 pooled explants was analysed by NanoString using a probe set containing recently identified31 and known PPR transcripts, otic markers and transcripts specific for other placodes as well as for the neural plate and neural crest, direct targets of various signalling pathways and housekeeping genes (see supplementary file 1).
The transcription factor Pax2, one of the earliest OEP-specific genes, is considered to be FGF dependent9,10,11, 15, 18, 20, 32,33,34,35,36,37,38,39,40. Surprisingly we find that its expression is activated at 12 hours, but subsequently lost (Fig. 1b–e; Supplementary Fig. S1, cluster 3). We verified this observation using in situ hybridisation: after 6 hours in vitro, Pax2 expression is not observed in isolated posterior PPR explants (n = 0/4 explants; Fig. 1b), but is clearly detectable at 12 hrs (5/8 explants; 62%; Fig. 1c,d), but not at 24 hrs (0/8 explants; Fig. 1e). Thus, Pax2 is transiently upregulated even in the absence of otic inducing signals. This observation prompted us to investigate whether other otic genes show a similar behaviour. We find that some otic transcripts like Etv5, PDL14, Axin2 and Sox9 behave similar to Pax2 with upwards trend at 12 hrs decreasing again at 24 hrs, while others like Eya1 and Sox10 are enhanced at 24 hours’ culture (Fig. 1f; note: not all changes are statistically significant). However, during the entire culture period lens and anterior transcripts (Pax6, Otx2, Dlx5, Dlx6; supplementary data 2) remain expressed at relatively high levels consistent with these explants being lens specified26. Although no FGFs are known to be expressed in the pPPR (see e.g. ref. 30), it is possible that placode progenitors have some residual FGF activity indicated by low levels of Etv5 expression at the time of explanting41, which however is not sufficient to complete otic induction. Together, these results suggest that posterior PPR cells may have an autonomous tendency to form OEPs, but do not realise this potential in the absence of additional signals.
A genetic hierarchy downstream of FGF signalling
In chick PPR explants, FGF2 mimics the activity of the endogenous OEP promoting signal, FGF199, 11, 14, 33, 42. To explore the dynamics in response to FGF signalling PPR explants (0 ss) freed from all surrounding tissues were cultured in the presence or absence of FGF2 for 6, 12 or 24 hours (Fig. 2a). Changes in the expression of 126 transcripts were quantified using NanoString (Supplementary File 2). To identify groups of genes with a similar FGF2-response profiles we performed hierarchical clustering of the log transformed gene expression levels (Supplementary Fig. S1) revealing 11 main clusters (denominated C1-C11). Transcripts in clusters C1, C5, C6 and C11 do not change in control or in FGF-treated conditions, while genes in other clusters are activated (C3, C7) or repressed (C10). These results indicate that FGF alone can only induce a small number of assayed transcripts, as also described previously23. Indeed, 6 hours of FGF exposure leads to the induction of only 6 transcripts (Fig. 2b) including the FGF target Etv5 41, the pPPR genes Foxi3 (Supplementary Fig. S2)43, Gbx2 (Supplementary Fig. S2)44 and Hey2 (Supplementary Fig. S2), the late otic gene Hesx1 45 (Supplementary Fig. S5) and the chemokine Cxcl14, which is normally expressed along the medial edge of the OEP domain (Supplementary Fig. S2). Except for Hey2 (cluster C2) these genes cluster together in C3. 12 hrs after FGF2 exposure genes normally expressed at otic placode stages are initiated (Znf217 [C6], Sall1 [C1]; Fig. 2c; Supplementary Fig. S1). Finally, after 24 hrs, Pax2 is significantly enhanced compared to controls together with a few signalling components (pNoc, BMP4, Fstl4; Supplementary Fig. S2) and chromatin remodelers (Chd7, Setd2; Fig. 2d; Supplementary Fig. S2).
While activating OEP associated genes, FGF exposure also leads to repression of genes normally absent from the otic territory. The majority of these transcripts fall into two clusters, C2 (Sstr5, Kremen1, Tox3, Ptpru and Gpr160) and C10 (Pax6, Dlx5/6 and Lef1) (Supplementary Fig. S1) and largely characterise the anterior PPR (future lens/olfactory; Supplementary Fig. S2)26, 30. This confirms the previous observation that FGF signalling is important to repress lens specification in non-lens ectoderm26. Finally, FGF also modulates other signalling pathways. While the WNT targets Lef1 (12 and 24 hrs) and Axin2 (12 hrs) are downregulated, the Notch target Hey2 46 increases. Likewise, FGF appears to modulate BMP signalling: the BMP antagonist Fstl4 is first repressed (6 hrs) and then induced (24 hrs) together with Bmp4 (Fig. 2b–d).
In summary, FGF signalling induces only a subset of the otic transcripts investigated here23 and does so in a temporal hierarchy. First, FGF enhances transcripts already expressed in the posterior PPR, followed by the initiation of OEP and late otic genes more downstream. At the same time, FGF activity ensures the repression of alternative fates.
FGF regulates Etv5 and Pax6 directly
Are all 6 hr-induced genes direct FGF targets? After 3 hrs of FGF2 treatment early OEP genes (Etv5, Cxcl14, Gbx2, Foxi3 and Pax2) are upregulated and lens genes (Pax6 and Sstr5) are repressed (Fig. 3b). To identify the direct targets, the same experiment was carried out in the presence of the translation inhibitor cycloheximide (CHX; Fig. 3a)47. Among the upregulated transcripts tested, only Etv5 appears as a direct FGF target (Fig. 3c), while Pax6 is the only factor repressed in the absence of protein synthesis (Fig. 3c). Therefore, the most parsimonious explanation for how FGF signalling activates the downstream network is that Etv5 regulates other upregulated factors, while Pax6 initiates the repressive cascade (Fig. 3d).
FGF activity is required for few mesoderm-induced OEP genes
In vivo, the head mesoderm is one of the FGF sources required for OEP induction33, 48. To investigate how the requirement for mesoderm-derived FGF changes over time we compared posterior PPR co-cultured with the head mesoderm in the presence of DMSO (control) or the FGFR inhibitor SU5402 (experimental; Fig. 4a) and assessed changes in gene expression after 6, 12 and 24 hrs using NanoString.
After 6 hours’ culture, 4 out of 6 mesoderm-induced transcripts depend on FGF signalling: the expression of Etv5, Foxi3, Hesx1, Cxcl14 is lost in the presence of the inhibitor (Fig. 4b). After 12 hrs another 6hr-induced gene, Gbx2, also emerges as FGF-dependent (Fig. 4c), while Hey2 induction is FGF independent. In addition, expression of the PPR genes Eya2 (6 hrs & 24 hrs; Fig. 4b,d) and Dlx6 (6 hrs; Fig. 4b) decreases in the presence of SU5402, suggesting that their maintenance requires FGF signalling. In contrast, repression of the anterior PPR genes tested is largely FGF independent and only Pax6 inhibition initially requires this pathway. Other anterior transcripts like Otx2, pNoc, Six3 and Sstr5 are decreased by mesodermal signals even when FGF signalling is reduced, as are Dlx5 and -6 at 24 hrs (Supplementary File 2).
After 12 and 24 hours’ culture other additional FGF-dependent factors emerge among them the otic placode genes Sox10 and Foxg1 (12 hrs; Fig. 4c) as well as Sox3, Zhx2 l and Homer2. Among the transcripts repressed by both the mesoderm and FGF, the non-neural ectoderm marker Gata2 together with epidermal Keratin19 stand out as the few genes whose repression after 12 hrs and 24 hrs, respectively, requires FGFR activity (Fig. 4c,d).
Together these results indicate that only those transcripts rapidly induced by FGF2 or the head mesoderm depend on FGF activity, while only a few late onset genes do. Likewise, repression of anterior character appears to be largely FGF independent, while inhibition of epidermal character may be mediated by FGF. Overall, these observations suggest that other signals must cooperate with mesoderm derived FGF to promote OEP specification.
Gene network inference and clustering identify sub-networks in the OEP programme
The above results reveal the molecular hierarchy downstream of FGF signalling as pPPR cells make the transition to OEPs. It is likely that direct FGF targets and early response genes (Etv5, Gbx2, Foxi3, Hey2) are at the top of this hierarchy providing input for late response genes. To explore this possibility in an unbiased way we used GENIE3, a Random Forest machine-learning algorithm, to infer a gene regulatory network (GRN) from the NanoString expression data. GENIE3 determines the importance of each factor within the network (regulator) in explaining the expression profile of a given target (by calculating importance measure: IM). To select an appropriate IM threshold the trade-off between recovery of true positives (based on data from the literature) and the number of overall predicted interactions was assessed (Fig. 5b); as the sensitivity of recovery drops, the threshold was set to 0.006. This results in a directed network of 3000 interactions and 109 nodes (Fig. 5a). To focus on the predictions with higher significance (larger IM values), the predicted interactions were ranked according to IM and the top 500 interactions were analysed in detail in Cytoscape (Fig. 5c; Supplementary File 3).
The predicted network topology reveals three modules termed M1, M2 and M3 (Fig. 5c) each containing genes with a similar response to FGF signalling: module M1 comprises genes repressed by FGF, many of which are normally expressed in the anterior PPR, module M2 contains early FGF response genes, while M3 includes factors regulated after 12 or 24 hours of FGF exposure. Node size in Fig. 5c indicates the centrality of each node within a module (see below).
To investigate the modularity of the emerging network, Newman’s community clustering was performed49 using the top 500 interactions of GENIE3 network (Supplementary File 3). This approach identifies gene hubs consisting of more connections within each hub than to the rest of the network. Five clusters (Newman’s cluster NC1-5) were identified consisting of 11 to 28 nodes and 19 to 92 edges (Fig. 6a, Supplementary Fig. S3); of these three clusters (NC1-3) correlate well with GENIE3 modules M1-M3 (see below). Both GENIE3 and Newmann’s community clustering predict groups of genes that may form a molecular sub-circuit and thus underlie a specific biological event (e.g. ‘early response to FGF’), however, they do not identify the most central genes in each circuit. We therefore calculated betweenness centrality for each node of the network as it provides a measure for the most connected nodes within a cluster (Fig. 5c). We displayed this in the GENIE3 network: large nodes show high betweenness centrality and are thus more central to the network. This analysis identifies four factors (Pax6, Dach1, Lef1 and Hesx1) as the most central nodes, as well as a larger number of slightly less well-connected nodes. These factors may play an important role during OEP specification in response to FGF signalling.
Finally, neither GENIE3 nor Newmann’s community clustering indicate whether the predicted interactions represent activation or repression of target genes. We therefore calculated Pearson’s correlation coefficient between all transcripts on the NanoString probe set (Fig. 6b: members of clusters NC1, NC2 and NC3 highlighted) assuming that positive correlations represent activating interactions, while negative correlations represent repressive interactions (Fig. 6a).
Next we examined the components of each cluster emerging from Newman’s community clustering and compared them to the GENIE3 modules. Cluster NC1 (Fig. 6a, NC1; Fig. 6b purple box) largely contains anterior PPR genes (Pax6, Sstr5, Nfkb1, Dlx5, Dlx6), similar to GENIE3 module M1. GO and KEGG term analysis (P-value < 0.05) reveals an enrichment of terms like anterior/posterior pattern formation, camera-type eye development and eye-photoreceptors. In agreement with this analysis, the eye ‘master regulator’ Pax6 emerges as the most central gene in cluster NC1 (Figs 5c and 6a), a notion that is further supported by its large number of predicted interactions (high out-degree).
The second cluster (Fig. 6a) resembles module M2 (Fig. 5c) comprising many OEP specific factors, which respond to FGF rapidly (e.g. 6 hrs: Etv5, Foxi3, Gbx2 and Hesx1). This cluster is therefore likely to represent the earliest phase of OEP induction. This is supported by the GO term analysis, which associates terms related to ear development and morphogenesis to this cluster (Fig. 6a).
Finally, the third cluster NC3 contains a mixture of genes (Fig. 6a), which characterise different tissues in the normal embryo, and overlaps with module M3 (Fig. 5c). It largely harbours late FGF response genes (12 or 24 hrs) including otic placode factors that are enhanced by FGF signalling (e.g. Bmp4, Hey2, Sall1, Sall4, Six4). In addition, NC3 also contains genes that are repressed by FGF (Lef1, Geminin, Sox9, Gata3, Sox10, Irx3, Zfhx1b and Zic1; Fig. 2b,d). Among these, Geminin, Zic1 and Zfhx1b are expressed in the neural plate, but absent from the otic territory50,51,52, while Sox9 and Sox10 are present in neural crest cells53, 54 and only later in the otic placode (Sox10). The canonical Wnt target Lef1 also is among the FGF-repressed genes. It not only emerges as a central node based on betweenness centrality, but with a high out-degree is predicted to regulate many targets. Indeed, the Wnt pathway regulates the transition from OEP to committed otic cells20, 55 and our model suggests that Lef1 is a key player during this process. In summary, NC3 may represent a module that promotes otic character, while at the same time repressing alternative fates.
The fourth and the fifth cluster (Supplementary Fig. S3) correspond to genes at the periphery of the GENIE3 network with very few interactions with the central nodes (Fig. 5c). Overall, this analysis indicates that using time-series data to model a GRN generates distinct modules that appear to recapitulate normal development during otic induction. In addition, this approach also reveals new factors hitherto not linked to ear formation that may play a central role during otic commitment.
Network predictions suggest new regulatory circuits to stabilise otic fate
The time course analysis described above reveals the genetic hierarchy downstream of FGF signalling as pPPR cells become specified as OEPs including both activated and repressed genes, while the GRN provides a global view of the network architecture that models this process. Our results reveal Etv5 and Pax6 as the only direct targets among the genes tested (Fig. 3), as well as a small cohort of transcripts whose expression is promoted or inhibited rapidly 6 hrs after FGF exposure (Fig. 2). Several of these have already been implicated in OEP specification (e.g. Foxi3, Gbx2, Six and Eya family members)8, 44 or in the acquisition of anterior placode fates (e.g. Pax6, SSTR5)30. However, how information is propagated through the network downstream of these factors to stabilise OEP identity and repress alternative fates is currently poorly understood. Here we use the predicted GRN to propose regulatory circuits by exploring the nearest neighbours of key FGF responsive genes and their predicted interactions.
Positive feedback loops stabilise the posterior PPR network downstream of FGF signalling
First, we briefly summarise the interactions of PPR and OEP transcription factors that have already been described. Members of the Six and Eya families are expressed in the entire PPR, while Foxi3 and Gbx2 are restricted to its posterior portion. Together, they provide crucial input for Pax2, one of the earliest genes labelling OEPs8, 56,57,58,59,60. Foxi1/3 and the Six1/Eya2 complex regulate each other in a positive feedback loop8, while Gbx2 is responsible to restrict Otx2 anteriorly44. Downstream of these factors FGF initiates OEP specification: the FGF mediators Etv4 and Etv5 become expressed41 and Pax2 expression is activated in response to FGF9,10,11, 15, 18, 20, 32,33,34,35, 37,38,39,40, 60 (Fig. 7a,a’).
Next we use our experimental time course and predictions to enrich the network upstream of Pax2 (Fig. 7b,b’). Of the genes tested, Etv5 emerges as the only direct FGF target in OEPs (Fig. 3). Our network therefore assumes that Etv5 regulates all FGF responsive genes as the simplest explanation. We also show that Foxi3 and Gbx2 are under the control of FGF (Figs 2 and 4) i.e. downstream of Etv5. Analysis of their nearest neighbours (Supplementary Fig. S4) predicts that all three factors promote the expression of the others, either directly (Etv5 ↔ Foxi3; Foxi3 ↔ Gbx2) or indirectly (Etv5 ↔ Gbx2 via Foxi3). Likewise, Etv5 and Eya2 are predicted to form a positive feedback loop (Supplementary Fig. S4) linking FGF input and the maintenance of the Six/Eya complex at PPR stages. Our finding that Eya2 maintenance requires FGF input (Fig. 4) supports this prediction. Finally, Pax2 is known to be regulated by Foxi3 and Gbx28, 44, 59, 62, 63, however our network analysis predicts that it is also activated directly by Etv5 (Supplementary Fig. S4). We therefore propose that a small circuit of positive feedback loops stabilises posterior PPR identity in response to FGF signalling (Fig. 7b’). Together FGF and the transcription factors within this circuit activate the OEP specific expression of Pax2 to initiate the otic programme.
Inhibitory loops refine gene expression in the otic placode
In the literature, few transcriptional interactions in the developing otic placode have been described. Foxg1 is regulated by FGF signalling23, while Pax2 has been reported to control the expression of Eya1 and Gata3 64. We show that prolonged FGF signalling (12 hrs) leads to the induction of a second set of genes (Foxg1, Hesx1, Sall1, Znf217), a time frame largely correlating well with their normal expression in the otic placode at 8–10 ss (Fig. 8). Hesx1, however, is normally only expressed at vesicle stages; thus FGF induces it prematurely in isolated explants. All four factors are transcriptional repressors65,66,67,68,69, which appear to initiate an inhibitory circuit that shuts down some early OEP genes and may limit the FGF response. Hesx1 is predicted to repress Eya2 and Foxi3 (Supplementary Fig. S4), which indeed are lost from the placode around the onset of Hesx1 in the otic vesicle43, 62, 70. Our data suggest that Hesx1 also represses Etv5, and thus may modulate FGF activity later (Fig. 8b; Supplementary Fig. S4). To test these predictions, we misexpressed Hesx1 in the otic territory at HH6 prior to its normal onset (Supplementary Fig. S5) and assessed the expression of Foxi3, Etv5 and Eya2 at 9–11 ss. We find that all three transcripts are indeed reduced (Fig. 8a–c; Foxi3: 2/5, Etv5: 2/11, Eya2: 2/10 embryos express normal levels).
The transcriptional repressor Sall1 is predicted to inhibit the PPR gene Six4 (Supplementary Fig. S4), whose otic expression declines over time, as well as the otic placode factor Sox10. Sox10 expression depends on FGF input (Fig. 4c), although FGF is not sufficient for its induction, and also requires Etv4, Sox8 and cMyb, which bind to its otic enhancer71. Thus, Sall1 may act to prevent its premature expression in response to these factors. Interestingly, both Six4 and Sox10 are predicted to enhance Sall1 expression thus forming a negative feedback loop (Supplementary Fig. S4, Fig. 8i).
Currently, nothing is known about the role of Znf217 in otic development. However, our predictions suggest that it is target of multiple repressive interactions from Sall1, Sox10 and the Wnt effector Lef1 (Supplementary Fig. S4, Fig. 8f). In summary, downstream of Pax2 and FGF, inhibitory loops appear to refine otic gene expression.
Repressing alternative fates via Pax2 and Foxg1
In the PPR precursors for different placodes are initially intermingled, but also mixed with future epidermal and neural crest cells. The mechanisms that segregate cells of different fates are only beginning to emerge. Gbx2 and Otx2 mutually repress each other to separate otic and epibranchial progenitors from more anterior placodes44. Likewise, FGF signalling initiates the repression of lens specification26 and we confirm this finding with our FGF time course analysis (Figs 2 and 4). In addition, other anterior transcripts are rapidly repressed by FGF signalling (Sstr5, Fstl4, GPR160, Ptpru) and we suggest that Foxg1 may play a central role to maintain their repressed state: Foxg1 is predicted to inhibit the expression of Sstr5 and Fstl4, as well as that of the lens/olfactory gene Six3 (Supplementary Fig. S4, Fig. 8h). Indeed, misexpression of Foxg1 in the anterior PPR inhibits Six3 expression (Fig. 8d; 3/15) confirming this prediction.
Likewise, several factors appear to cooperate to prevent epidermal gene expression. FGF inhibits epidermal Keratin19 and Gata2, and this pathway is indeed required for their absence from otic cells (Figs 2 and 4). In addition, our network suggests that FGF acts through Foxg1 and Pax2 to repress Gata2, while conversely Gata2 is predicted to repress Pax2, Foxg1, Gbx2 and Etv5 (Supplementary Fig. S4, Fig. 8f). Thus, preventing Gata2 expression appears crucial to allow otic placode formation.
FGF signalling prevents premature activation of canonical Wnt signalling
While FGF activity is required for OEP induction, it must be switched off for cells to mature and acquire otic identity. Thereafter, canonical Wnt signalling promotes otic commitment20, 22, 55. Our data suggest that FGF plays a role in preventing premature activation of the Wnt pathway. Axin2, a readout for canonical Wnt activity, is rapidly upregulated when FGF is inhibited, and actively repressed after prolonged FGF exposure (Figs 2 and 4) as are Lef1 and the Wnt co-receptor Kremen1. Our network analysis proposes that Foxi3 mediates FGF action, since it is predicted to repress Lef1. Conversely, Lef1 itself is predicted to inhibit several FGF dependent otic genes including Foxg1, Gbx2 and Znf217, which are normally expressed before Wnt signalling becomes active in the otic placode (Supplementary Fig. S4, Fig. 8f). These results highlight how different signals modulate each other’s activity to control otic development and point to the regulatory circuits mediating this process.
Discussion
The vertebrate inner ear arises from a pool of sensory progenitor cells that are initially competent to contribute to all sense organs and sensory ganglia in the head. Over time their potential is restricted, and cells next to the hindbrain become committed to the ear lineage. Rather than involving a single molecular switch ear commitment is achieved gradually as cells are exposed to different sequential signals1, 28, 29. FGF signalling is widely accepted as otic inducing signal: in the absence of FGF activity the otic placode does not form10, 11, 15, 17, 18, 23, 32, 34, 40, 42, 72,73,74,75,76,77,78 and when exposed to FGFs placode progenitors activate the otic-epibranchial programme15, 32, 37,38,39,40, 77, 79,80,81. Here we dissect the temporal hierarchy downstream of FGF signalling using a combination of experimental and network inference approaches. Our findings suggest that the main role of FGF during otic-epibranchial progenitor induction is to activate a small transcriptional circuit, which in turn may be sufficient to implement the ear programme autonomously.
Analysing the response of sensory progenitors to FGF over time reveals that rather than inducing many genes, FGF rapidly promotes the expression of a few transcription factors (Etv5, Foxi3 and Gbx2), while others are initiated much later. Etv5 appears to be the only direct FGF target of the genes tested placing Foxi3 and Gbx2 downstream of Etv5. All three factors are already expressed in sensory progenitors: FGF enhances, but does not induce their expression. It is possible that posterior PPR cells retain residual FGF activity and this may explain the transient upregulation of otic genes in vitro, in the absence of exogenous FGFs (Fig. 1). Network predictions indicate that Etv5, Foxi3 and Gbx2 perpetuate their own expression thus locking cells in a posterior PPR transcriptional state (Fig. 7b’). Foxi3 also forms a positive feedback loop with the PPR specifiers Six1 and Eya28, 62, 82, and together they regulate the onset of Pax2, the earliest known OEP marker8, 57, 58, 62, 63, 77, 80, 83, 84. Together, our data suggest that once this circuit of positive feedback loops is established, cells are able to maintain their identity even in the absence of FGF signalling (Fig. 7b’). Indeed, OEPs are specified as soon as Pax2 becomes expressed (4–5 ss): when cultured in isolation OEP explants continue to express otic specific genes and generate neurons in the absence of additional signals24, 25. We therefore suggest that the major role of FGF signalling during otic placode initiation is to activate a small sub-circuit of genes, whose role is to stabilise the OEP programme before additional signals commit cells to inner ear or epibranchial identity.
FGFs are critical to activate the OEP programme. However, it has been suggested that attenuation of the pathway is required for cells to become committed to the ear lineage, while continued signalling is necessary for epibranchial placodes to form12, 16, 20. Thus, FGF signalling may be tightly controlled and this may occur on multiple levels. Sprouty1 and -2 inhibit MAPK signalling downstream of the FGF receptor85, 86 and both become rapidly upregulated as the placode forms87,88,89. In their absence, the otic placode is enlarged and cells that normally contribute to the epidermis are now recruited into the placode suggesting that FGF inhibition is required to control otic placode size87. Our network analysis points to a second mechanism to regulate FGF signalling acting at vesicle stages. Downstream of the early OEP circuit, several transcriptional repressors are activated including Hesx1 65, 66, 69. We show that when expressed prematurely, Hesx1 represses the transcription factor Etv5, a direct target of FGF signalling (Fig. 8b) suggesting a possible role in limiting FGF signalling in the otic vesicle.
Having received FGF signalling OEPs are rapidly specified25 becoming independent of additional signals suggesting that transcriptional programmes must be in place to segregate otic cells from other ectodermal fates and to reinforce ear identity. Our network analysis and functional experiments demonstrate that Hesx1 not only represses Etv5, but also the posterior PPR genes Foxi3 and Eya2. Indeed, both are downregulated as the otic placode matures and it is possible that this is required to maintain otic character. Likewise, the transcriptional repressor Foxg1 is activated downstream of the OEP network. Network inference predicts Foxg1 to be key for repression of other fates (Fig. 8h), in particular anterior PPR derivatives like lens and olfactory placodes. We have previously shown that lens is the default state of all sensory progenitors and that FGF signalling initiates, but does not complete lens repression in non-lens ectoderm26. Here we show that the lens transcription factor Pax6 is a direct target of FGF signalling and propose that Foxg1 continues to prevent its activation in the ear. Our network analysis predicts that Foxg1 represses two different Pax6 regulators: the somatostatin receptor SSTR5 30 and the transcription factor Six3 which binds to the Pax6-lens enhancer90, and our functional data confirm Six3 repression by Foxg1. Together, our data suggest that repressive loops are critical to ensure the progression of OEPs towards otic commitment, while simultaneously preventing alternative fates.
In summary, using a combination of time course analysis and network inference we describe a framework for understanding the regulatory logic that initiates ear development from sensory progenitors. Our gene network highlights the hierarchical organisation of otic induction and provides mechanistic insight into how signalling information is propagated through the network. We suggest that downstream of FGF signalling a few transcription factors form a circuit of positive feedback loops that is sufficient to maintain OEP identity and thus keeps cells competent to respond to the next signalling input.
Methods
All experiments were carried out in accordance with the institutional guidelines and regulations.
Embryo manipulation and pPPR explant culture
Experiments on chick embryos prior to E10 do not require a home office license or institutional approval and were carried out according to the institutional guidelines. Fertilized hens’ eggs were obtained from Winter Farm (Herts, UK) and incubated in a humidified incubator at 38 °C hours until reaching primitive streak or head fold stages. For culture, embryos were isolated using filter papers91, electroporated using 5 pulses of 4.7 V for 50 ms each with a 750 ms gap as previously described92 and maintained in filter paper culture until they had reached 9–12 ss. Foxg1overexpression was carried out at primitive streak stages and Hesx1 overexpression at head fold stages. For explant cultures, head fold stage embryos were isolated in Tyrode’s saline; the pPPR ectoderm with or without the underlying mesoderm were dissected and then cultured in collagen drops as described26. Culture medium and collagen were supplemented with FGF2 (0.25ng/μl; R&D), DMSO, SU5402 (10 μM; Tocris) or CHX (10 μM; Sigma). Tissues were cultured for 3, 6, 12 and 24 hours.
NanoString nCounter
A NanoString probe set (Supplementary File 1) was designed containing known otic and other placode markers, known PPR, neural, neural crest and non-neural ectoderm markers and new placode genes identified in a recent microarray screen for new regulators in placode formation (unpublished). For each experimental condition, eight to ten explants were lysed in 5 μl of lysis buffer (Ambion). For each condition three independent experiments were carried out and analyzed by nCounter® Analysis System (Life Sciences) using a customized probe set of 126 genes. Total RNA was hybridized with capture and reporter probes at 65 °C over night. According to the nCounter Gene Expression Assay Manual the target/probe complexes were washed, immobilized, and data were collected by the nCounter Digital Analyzer. Data were analyzed following company instructions. A cut off of fold change >= 1.25 and <= 0.75 was used to identify upregulated and downregulated genes, respectively, in combination with a p-value <=0.05 (unpaired t-test). Full list of probes and their targeted sequences are in Supplementary File 1.
Plasmids, antibodies and in situ hybridization
The following chick ESTs were used to generate Digoxigenin–labeled antisense probes: Chd7 ChEST757h23, Cxcl14 ChEST896P24, Fstl4 ChEST433o1, GPR160 ChEST21c16, Hey2 ChEST923p18, Homer2 ChEST795g2, Kremen1-like ChEST751a10, Mynn ChEST536f8, PTPRU ChEST714k5 and Tox3 ChEST1009p6. Etv5 was obtained from M. Bronner, Foxi3 from A. Groves, Gata2 and Lef1 from C.D. Stern, Pax2 from M. Golding and Pax6 from A. Bang. RNA probes were synthesized with T7, T3 or SP6 RNA polymerase (Roche). Whole mount or explant in situ hybridization was performed as described previously93. Mouse Foxg1 (a gift from C. Houart) and Hesx1 (a gift form J.P. Barbera-Martinez) were co-electroporated with eGFP. Electroporated embryos were processed for in situ hybridization followed by antibody staining for GFP (Invitrogen) using an HRP-coupled secondary antibody (Jackson) as previously described92, 93.
Gene regulatory network (GRN) inference
GRN inference of the normalised NanoString data was carried out using GENIE3 R implementation. GENIE3 outperforms other popular inference methods on real and simulated data94 and shows excellent performance in previous studies95, 96. Before network inference, genes with very low expression values (<0.00004), which cannot be detected by in situ hybridization, were treated as absent and their values set to 0. As GENIE3 input, the normalised NanoString gene expression data and a list of transcription factors (potential regulators in the NanoString dataset) were used. GENIE3 produces a directed network by attempting to explain the expression profile of a target gene by the expression profiles of all input genes using a tree-based ensemble method: Random Forests. Then the importance of each input gene (regulator) in explaining the expression profile of a target gene is calculated by inferring a network n number of times (n = 1000 used in present study). The importance measure (IM) is then taken as an indication of a putative regulatory link. Following network inference, all regulatory links were ranked according to their IM with larger values indicating greater significance. To test the efficacy of the network, the predicted interactions were compared to 76 known interactions from the literature between PPR to otic placode stages using union and intersection functions in Cytoscape. After assessing the percentage of true positives retrieved (sensitivity) against the total number of predicted interactions, a threshold of 0.006 on the IM was considered optimal.
Clustering
To identify groups of co-expressed genes in the NanoString data, normalised expression values of genes were used to perform hierarchical clustering (using Euclidean distance) and to generate heatmaps using the R package gplots97. To identify modules in the network, Community clustering49 was performed using the GLay plugin98 in Cytoscape. The advantage of Girvan and Newman’s clustering algorithm is that it does not require the number of clusters to be fixed as in other clustering techniques such as K-means. Thus, it allows finding the natural community structure within the network. Following clustering, the resulting modules were annotated with Gene Ontology (GO) and KEGG pathways using Cytoscape plugin BiNGO99, 100.
Correlation analysis
To determine negative and positive relationships in GENIE3 predicted network, Pearson’s correlation coefficient was calculated between all pairs of genes in the NanoString data and displayed as a heatmap using the R package gplots97.
Network display
The network was viewed and analysed in Cytoscape v 3.0.2101. Size and colour of the nodes were assigned according to the betweenness centrality (number of shortest paths between nodes in the network that pass through a particular node) or out-degree of each node in the network and the edges were weighted according to the IM values. The gene regulatory network models were drawn using BioTapestry102,103,104.
References
Chen, J. & Streit, A. Induction of the inner ear: stepwise specification of otic fate from multipotent progenitors. Hearing Research 297, 3–12 (2013).
Sai, X. & Ladher, R. K. Early steps in inner ear development: induction and morphogenesis of the otic placode. Front Pharmacol 6, 19 (2015).
Bhattacharyya, S., Bailey, A. P., Bronner-Fraser, M. & Streit, A. Segregation of lens and olfactory precursors from a common territory: cell sorting and reciprocity of Dlx5 and Pax6 expression. Developmental Biology 271, 403–414 (2004).
Kozlowski, D. J., Murakami, T., Ho, R. K. & Weinberg, E. S. Regional cell movement and tissue patterning in the zebrafish embryo revealed by fate mapping with caged fluorescein. Biochemistry and Cell Biology 75, 551–562 (1997).
Pieper, M., Eagleson, G. W., Wosniok, W. & Schlosser, G. Origin and segregation of cranial placodes in Xenopus laevis. Developmental Biology 360, 257–275 (2011).
Streit, A. Extensive Cell Movements Accompany Formation of the Otic Placode. Developmental Biology 249, 237–254 (2002).
Xu, X., Dude, C. M. & Baker, C. V. Fine-grained fate maps for the ophthalmic and maxillomandibular trigeminal placodes in the chick embryo. Developmental Biology 317, 174–186 (2008).
Khatri, S. B., Edlund, R. K. & Groves, A. K. Foxi3 is necessary for the induction of the chick otic placode in response to FGF signaling. Developmental Biology 391, 158–169 (2014).
Ladher, R. K., Anakwe, K. U., Gurney, A. L., Schoenwolf, G. C. & Francis-West, P. H. Identification of synergistic signals initiating inner ear development. Science 290, 1965–1967 (2000).
Maroon, H. et al. Fgf3 and Fgf8 are required together for formation of the otic placode and vesicle. Development 129, 2099–2108 (2002).
Martin, K. & Groves, A. K. Competence of cranial ectoderm to respond to Fgf signaling suggests a two-step model of otic placode induction. Development 133, 877–887 (2006).
Nechiporuk, A., Linbo, T., Poss, K. D. & Raible, D. W. Specification of epibranchial placodes in zebrafish. Development 134, 611–623 (2007).
Nikaido, M. et al. Initial specification of the epibranchial placode in zebrafish embryos depends on the fibroblast growth factor signal. Developmental Dynamics 236, 564–571 (2007).
Paxton, C. N., Bleyl, S. B., Chapman, S. C. & Schoenwolf, G. C. Identification of differentially expressed genes in early inner ear development. Gene expression patterns: GEP 10, 31–43 (2010).
Phillips, B. T., Bolding, K. & Riley, B. B. Zebrafish fgf3 and fgf8 encode redundant functions required for otic placode induction. Developmental Biology 235, 351–365 (2001).
Sun, S. K. et al. Epibranchial and otic placodes are induced by a common Fgf signal, but their subsequent development is independent. Developmental Biology 303, 675–686 (2007).
Urness, L. D., Paxton, C. N., Wang, X., Schoenwolf, G. C. & Mansour, S. L. FGF signaling regulates otic placode induction and refinement by controlling both ectodermal target genes and hindbrain Wnt8a. Developmental Biology 340, 595–604 (2010).
Wright, T. J. & Mansour, S. L. Fgf3 and Fgf10 are required for mouse otic placode induction. Development 130, 3379–3390 (2003).
Yang, J., Ellinor, P. T., Sather, W. A., Zhang, J. F. & Tsien, R. W. Molecular determinants of Ca2+ selectivity and ion permeation in L-type Ca2+ channels. Nature 366, 158–161 (1993).
Freter, S., Muta, Y., Mak, S. S., Rinkwitz, S. & Ladher, R. K. Progressive restriction of otic fate: the role of FGF and Wnt in resolving inner ear potential. Development 135, 3415–3424 (2008).
Jayasena, C. S., Ohyama, T., Segil, N. & Groves, A. K. Notch signaling augments the canonical Wnt pathway to specify the size of the otic placode. Development 135, 2251–2261 (2008).
Ohyama, T., Mohamed, O. A., Taketo, M. M., Dufort, D. & Groves, A. K. Wnt signals mediate a fate decision between otic placode and epidermis. Development 133, 865–875 (2006).
Yang, L. et al. Analysis of FGF-dependent and FGF-independent pathways in otic placode induction. PloS one 8, e55011 (2013).
Adam, J. et al. Cell fate choices and the expression of Notch, Delta and Serrate homologues in the chick inner ear: parallels with Drosophila sense-organ development. Development 125, 4645–4654 (1998).
Groves, A. K. & Bronner-Fraser, M. Competence, specification and commitment in otic placode induction. Development 127, 3489–3499 (2000).
Bailey, A. P., Bhattacharyya, S., Bronner-Fraser, M. & Streit, A. Lens specification is the ground state of all sensory placodes, from which FGF promotes olfactory identity. Dev Cell 11, 505–517 (2006).
Grocott, T., Tambalo, M. & Streit, A. The peripheral sensory nervous system in the vertebrate head: a gene regulatory perspective. Developmental Biology 370, 3–23 (2012).
Ladher, R. K., O’Neill, P. & Begbie, J. From shared lineage to distinct functions: the development of the inner ear and epibranchial placodes. Development 137, 1777–1785 (2010).
Ohyama, T., Groves, A. K. & Martin, K. The first steps towards hearing: mechanisms of otic placode induction. The International Journal of Developmental Biology 51, 463–472 (2007).
Lleras-Forero, L. et al. Neuropeptides: developmental signals in placode progenitor formation. Dev Cell 26, 195–203 (2013).
Hintze, M. et al. Cell interactions, singals and transcriptional hierarchy governing placode progenitor induction. Development, in press, (2017).
Alvarez, Y. et al. Requirements for FGF3 and FGF10 during inner ear formation. Development 130, 6329–6338 (2003).
Kil, S. H. et al. Distinct roles for hindbrain and paraxial mesoderm in the induction and patterning of the inner ear revealed by a study of vitamin-A-deficient quail. Developmental Biology 285, 252–271 (2005).
Leger, S. & Brand, M. Fgf8 and Fgf3 are required for zebrafish ear placode induction, maintenance and inner ear patterning. Mechanisms of Development 119, 91–108 (2002).
Mansour, S. L. Targeted disruption of int-2 (fgf-3) causes developmental defects in the tail and inner ear. Molecular reproduction and development 39, 62–67, discussion 67–68 (1994).
Ohuchi, H. et al. FGF10 acts as a major ligand for FGF receptor 2 IIIb in mouse multi-organ development. Biochemical and biophysical research communications 277, 643–649 (2000).
Padanad, M. S., Bhat, N., Guo, B. & Riley, B. B. Conditions that influence the response to Fgf during otic placode induction. Developmental Biology 364, 1–10 (2012).
Phillips, B. T., Storch, E. M., Lekven, A. C. & Riley, B. B. A direct role for Fgf but not Wnt in otic placode induction. Development 131, 923–931 (2004).
Vendrell, V., Carnicero, E., Giraldez, F., Alonso, M. T. & Schimmang, T. Induction of inner ear fate by FGF3. Development 127, 2011–2019 (2000).
Zelarayan, L. C. et al. Differential requirements for FGF3, FGF8 and FGF10 during inner ear development. Developmental Biology 308, 379–391 (2007).
Lunn, J. S., Fishwick, K. J., Halley, P. A. & Storey, K. G. A spatial and temporal map of FGF/Erk1/2 activity and response repertoires in the early chick embryo. Developmental Biology 302, 536–552 (2007).
Ladher, R. K., Wright, T. J., Moon, A. M., Mansour, S. L. & Schoenwolf, G. C. FGF8 initiates inner ear induction in chick and mouse. Genes & Development 19, 603–613 (2005).
Khatri, S. B. & Groves, A. K. Expression of the Foxi2 and Foxi3 transcription factors during development of chicken sensory placodes and pharyngeal arches. Gene expression patterns: GEP 13, 38–42 (2013).
Steventon, B., Mayor, R. & Streit, A. Mutual repression between Gbx2 and Otx2 in sensory placodes reveals a general mechanism for ectodermal patterning. Developmental Biology 367, 55–65 (2012).
Abe, Y., Chen, W., Huang, W., Nishino, M. & Li, Y. P. CNBP regulates forebrain formation at organogenesis stage in chick embryos. Developmental Biology 295, 116–127 (2006).
Doetzlhofer, A. et al. Hey2 regulation by FGF provides a Notch-independent mechanism for maintaining pillar cell fate in the organ of Corti. Dev Cell 16, 58–69 (2009).
Palmeirim, I., Henrique, D., Ish-Horowicz, D. & Pourquie, O. Avian hairy gene expression identifies a molecular clock linked to vertebrate segmentation and somitogenesis. Cell 91, 639–648 (1997).
Orts, F., Jimenez-Collado, L. & Jimenez-Collado, J. Regulation of the embryo after the extirpation of Hensen’s node. Consequences on the differentiation of the otic placode. Archives d’anatomie, d’histologie et d’embryologie normales et experimentales 54, 1–11 (1971).
Newman, M. E. & Girvan, M. Finding and evaluating community structure in networks. Physical review. E, Statistical, nonlinear, and soft matter physics 69, 026113 (2004).
Dady, A., Blavet, C. & Duband, J. L. Timing and kinetics of E- to N-cadherin switch during neurulation in the avian embryo. Developmental Dynamics 241, 1333–1349 (2012).
Khudyakov, J. & Bronner-Fraser, M. Comprehensive spatiotemporal analysis of early chick neural crest network genes. Developmental Dynamics 238, 716–723 (2009).
Papanayotou, C. et al. A mechanism regulating the onset of Sox2 expression in the embryonic neural plate. PLoS Biology 6, e2 (2008).
Betancur, P., Bronner-Fraser, M. & Sauka-Spengler, T. Genomic code for Sox10 activation reveals a key regulatory enhancer for cranial neural crest. PNAS 107, 3570–3575 (2010).
McKeown, S. J., Lee, V. M., Bronner-Fraser, M., Newgreen, D. F. & Farlie, P. G. Sox10 overexpression induces neural crest-like cells from all dorsoventral levels of the neural tube but inhibits differentiation. Developmental dynamics 233, 430–444 (2005).
McCarroll, M. N. et al. Graded levels of Pax2a and Pax8 regulate cell differentiation during sensory placode formation. Development 139, 2740–2750 (2012).
Brugmann, S. A., Pandur, P. D., Kenyon, K. L., Pignoni, F. & Moody, S. A. Six1 promotes a placodal fate within the lateral neurogenic ectoderm by functioning as both a transcriptional activator and repressor. Development 131, 5871–5881 (2004).
Christophorou, N. A., Bailey, A. P., Hanson, S. & Streit, A. Activation of Six1 target genes is required for sensory placode formation. Developmental Biology 336, 327–336 (2009).
Hans, S., Liu, D. & Westerfield, M. Pax8 and Pax2a function synergistically in otic specification, downstream of the Foxi1 and Dlx3b transcription factors. Development 131, 5091–5102 (2004).
Nissen, R. M. Zebrafish foxi one modulates cellular responses to Fgf signaling required for the integrity of ear and jaw patterning. Development 130, 2543–2554 (2003).
Solomon, K. S., Logsdon, J. M. Jr. & Fritz, A. Expression and phylogenetic analyses of three zebrafish FoxI class genes. Developmental dynamics 228, 301–307 (2003).
Ohuchi, H., Kimura, S., Watamoto, M. & Itoh, N. Involvement of fibroblast growth factor (FGF)18-FGF8 signaling in specification of left-right asymmetry and brain and limb development of the chick embryo. Mechanisms of Development 95, 55–66 (2000).
Birol, O. et al. The mouse Foxi3 transcription factor is necessary for the development of posterior placodes. Developmental Biology 409, 139–151 (2016).
Bricaud, O. & Collazo, A. The transcription factor six1 inhibits neuronal and promotes hair cell fate in the developing zebrafish (Danio rerio) inner ear. The Journal of Neuroscience 26, 10438–10451 (2006).
Christophorou, N. A., Mende, M., Lleras-Forero, L., Grocott, T. & Streit, A. Pax2 coordinates epithelial morphogenesis and cell fate in the inner ear. Developmental Biology 345, 180–190 (2010).
Brickman, J. M. et al. Molecular effects of novel mutations in Hesx1/HESX1 associated with human pituitary disorders. Development 128, 5189–5199 (2001).
Carvalho, L. R. et al. A homozygous mutation in HESX1 is associated with evolving hypopituitarism due to impaired repressor-corepressor interaction. The Journal of clinical investigation 112, 1192–1201 (2003).
Cowger, J. J., Zhao, Q., Isovic, M. & Torchia, J. Biochemical characterization of the zinc-finger protein 217 transcriptional repressor complex: identification of a ZNF217 consensus recognition sequence. Oncogene 26, 3378–3386 (2007).
Netzer, C. et al. SALL1, the gene mutated in Townes-Brocks syndrome, encodes a transcriptional repressor which interacts with TRF1/PIN2 and localizes to pericentromeric heterochromatin. Human molecular genetics 10, 3017–3024 (2001).
Yao, J., Lai, E. & Stifani, S. The winged-helix protein brain factor 1 interacts with groucho and hes proteins to repress transcription. Molecular and Cellular Biology 21, 1962–1972 (2001).
Ishihara, T., Ikeda, K., Sato, S., Yajima, H. & Kawakami, K. Differential expression of Eya1 and Eya2 during chick early embryonic development. Gene expression patterns: GEP 8, 357–367 (2008).
Betancur, P., Sauka-Spengler, T. & Bronner, M. A Sox10 enhancer element common to the otic placode and neural crest is activated by tissue-specific paralogs. Development 138, 3689–3698 (2011).
Abello, G. et al. Independent regulation of Sox3 and Lmx1b by FGF and BMP signaling influences the neurogenic and non-neurogenic domains in the chick otic placode. Developmental Biology 339, 166–178 (2010).
Liu, D. et al. Fgf3 and Fgf8 dependent and independent transcription factors are required for otic placode specification. Development 130, 2213–2224 (2003).
Maulding, K., Padanad, M. S., Dong, J. & Riley, B. B. Mesodermal Fgf10b cooperates with other Fgfs during induction of otic and epibranchial placodes in zebrafish. Developmental dynamics 243 (2014).
Meyers, E. N., Lewandoski, M. & Martin, G. R. An Fgf8 mutant allelic series generated by Cre- and Flp-mediated recombination. Nature Genetics 18, 136–141 (1998).
Pirvola, U. et al. FGF/FGFR-2(IIIb) signaling is essential for inner ear morphogenesis. The Journal of neuroscience: the official journal of the Society for Neuroscience 20, 6125–6134 (2000).
Solomon, K. S., Kwak, S. J. & Fritz, A. Genetic interactions underlying otic placode induction and formation. Developmental dynamics 230, 419–433 (2004).
Tekin, M., Arnos, K. S. & Pandya, A. Advances in hereditary deafness. Lancet 358, 1082–1090 (2001).
Bajoghli, B., Aghaallaei, N., Heimbucher, T. & Czerny, T. An artificial promoter construct for heat-inducible misexpression during fish embryogenesis. Developmental Biology 271, 416–430 (2004).
Hans, S., Christison, J., Liu, D. & Westerfield, M. Fgf-dependent otic induction requires competence provided by Foxi1 and Dlx3b. BMC Dev Biol 7, 5 (2007).
Lombardo, A., Isaacs, H. V. & Slack, J. M. Expression and functions of FGF-3 in Xenopus development. The International Journal of Developmental Biology 42, 1101–1107 (1998).
Kwon, H. J., Bhat, N., Sweet, E. M., Cornell, R. A. & Riley, B. B. Identification of early requirements for preplacodal ectoderm and sensory organ development. PLoS Genetics 6, e1001133 (2010).
Mackereth, M. D., Kwak, S. J., Fritz, A. & Riley, B. B. Zebrafish pax8 is required for otic placode induction and plays a redundant role with Pax2 genes in the maintenance of the otic placode. Development 132, 371–382 (2005).
Padanad, M. S. & Riley, B. B. Pax2/8 proteins coordinate sequential induction of otic and epibranchial placodes through differential regulation of foxi1, sox3 and fgf24. Developmental Biology 351, 90–98 (2011).
Hacohen, N., Kramer, S., Sutherland, D., Hiromi, Y. & Krasnow, M. A. sprouty encodes a novel antagonist of FGF signaling that patterns apical branching of the Drosophila airways. Cell 92, 253–263 (1998).
Yusoff, P. et al. Sprouty2 inhibits the Ras/MAP kinase pathway by inhibiting the activation of Raf. The Journal of Biological Chemistry 277, 3195–3201 (2002).
Rogers, A. A. M., Zhang, J. & Shim, K. Sprouty1 and Sprouty2 limit both the size of the otic placode and hindbrain Wnt8a by antagonizing FGF signaling. Developmental Biology 353, 94–104 (2011).
Wright, K. D., Mahoney Rogers, A. A., Zhang, J. & Shim, K. Cooperative and independent functions of FGF and Wnt signaling during early inner ear development. BMC Dev Biol 15, 33 (2015).
Zhang, J., Wright, K. D., Mahoney Rogers, A. A., Barrett, M. M. & Shim, K. Compensatory regulation of the size of the inner ear in response to excess induction of otic progenitors by fibroblast growth factor signaling. Developmental dynamics 243, 1317–1327 (2014).
Liu, W., Lagutin, O. V., Mende, M., Streit, A. & Oliver, G. Six3 activation of Pax6 expression is essential for mammalian lens induction and specification. The EMBO journal 25, 5383–5395 (2006).
Streit, A. EC culture: a method to culture early chick embryos. Methods in Molecular Biology 461, 255–264 (2008).
Norris, A. & Streit, A. Morpholinos: studying gene function in the chick. Methods 66, 454–465 (2014).
Streit, A. & Stern, C. D. Combined whole-mount in situ hybridization and immunohistochemistry in avian embryos. Methods 23, 339–344 (2001).
Huynh-Thu, V. A., Irrthum, A., Wehenkel, L. & Geurts, P. Inferring regulatory networks from expression data using tree-based methods. PloS one 5 (2010).
Omranian, N., Eloundou-Mbebi, J. M., Mueller-Roeber, B. & Nikoloski, Z. Gene regulatory network inference using fused LASSO on multiple data sets. Scientific reports 6, 20533 (2016).
Potier, D. et al. Mapping gene regulatory networks in Drosophila eye development by large-scale transcriptome perturbations and motif inference. Cell Rep 9, 2290–2303 (2014).
Warnes, G. R. et al. Gplots: Various R programming tools for plotting data (2015).
Su, G., Kuchinsky, A., Morris, J. H., States, D. J. & Meng, F. GLay: community structure analysis of biological networks. Bioinformatics 26, 3135–3137 (2010).
Bindea, G. et al. ClueGO: a Cytoscape plug-in to decipher functionally grouped gene ontology and pathway annotation networks. Bioinformatics 25, 1091–1093 (2009).
Maere, S., Heymans, K. & Kuiper, M. BiNGO: a Cytoscape plugin to assess overrepresentation of gene ontology categories in biological networks. Bioinformatics 21, 3448–3449 (2005).
Shannon, P. et al. Cytoscape: a software environment for integrated models of biomolecular interaction networks. Genome research 13, 2498–2504 (2003).
Longabaugh, W. J., Davidson, E. H. & Bolouri, H. Computational representation of developmental genetic regulatory networks. Developmental Biology 283, 1–16 (2005).
Longabaugh, W. J., Davidson, E. H. & Bolouri, H. Visualization, documentation, analysis, and communication of large-scale gene regulatory networks. Biochim Biophys Acta 1789, 363–374 (2009).
Paquette, S. M., Leinonen, K. & Longabaugh, W. J. BioTapestry now provides a web application and improved drawing and layout tools. F1000Res 5, 39 (2016).
Acknowledgements
The authors thank Ewa Kolano for excellent technical assistance and Claudio D. Stern for critical reading of the manuscript. This work was supported by a studentship grant from Deafness Research UK (now Action on Hearing Loss; 513:KCL:AS) to A.S., and project grants to A.S. by the BBSCR BB/I021647/1, Wellcome Trust (081531/Z/06/Z) and NIH (NIDCD 1R01DC011577-01A1) and an international studentship from King’s College London to M.A.
Author information
Authors and Affiliations
Contributions
M.A. performed and analysed all network inference and clustering approaches, contributed to in situ hybridisation analysis and prepared figures; M.T. performed and analysed most wet-lab experiments; R.R. performed and analysed all electroporation experiments; T.G. contributed to explant experiments, in situ hybridisation and the selection of genes for NanoString; A.S. conceived the project and together with M.A. and M.T. designed and interpreted the experiments; A.S. wrote the manuscript together with M.A. and M.T. All authors reviewed the manuscript.
Corresponding author
Ethics declarations
Competing Interests
The authors declare that they have no competing interests.
Additional information
Publisher's note: Springer Nature remains neutral with regard to jurisdictional claims in published maps and institutional affiliations.
Electronic supplementary material
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/.
About this article
Cite this article
Anwar, M., Tambalo, M., Ranganathan, R. et al. A gene network regulated by FGF signalling during ear development. Sci Rep 7, 6162 (2017). https://doi.org/10.1038/s41598-017-05472-0
Received:
Accepted:
Published:
DOI: https://doi.org/10.1038/s41598-017-05472-0
This article is cited by
-
FOXI3 pathogenic variants cause one form of craniofacial microsomia
Nature Communications (2023)
-
Inferring and analyzing gene regulatory networks from multi-factorial expression data: a complete and interactive suite
BMC Genomics (2021)
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.