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A novel gene’s role in an ancient mechanism: secreted Frizzled-related protein 1 is a critical component in the anterior–posterior Wnt signaling network that governs the establishment of the anterior neuroectoderm in sea urchin embryos

EvoDevo20189:1

https://doi.org/10.1186/s13227-017-0089-3

  • Received: 15 October 2017
  • Accepted: 18 December 2017
  • Published:

Abstract

The anterior neuroectoderm (ANE) in many deuterostome embryos (echinoderms, hemichordates, urochordates, cephalochordates, and vertebrates) is progressively restricted along the anterior–posterior axis to a domain around the anterior pole. In the sea urchin embryo, three integrated Wnt signaling branches (Wnt/β-catenin, Wnt/JNK, and Wnt/PKC) govern this progressive restriction process, which begins around the 32- to 60-cell stage and terminates by the early gastrula stage. We previously have established that several secreted Wnt modulators of the Dickkopf and secreted Frizzled-related protein families (Dkk1, Dkk3, and sFRP-1/5) are expressed within the ANE and play important roles in modulating the Wnt signaling network during this process. In this study, we use morpholino and dominant-negative interference approaches to characterize the function of a novel Frizzled-related protein, secreted Frizzled-related protein 1 (sFRP-1), during ANE restriction. sFRP-1 appears to be related to a secreted Wnt modulator, sFRP3/4, that is essential to block Wnt signaling and establish the ANE in vertebrates. Here, we show that the sea urchin sFRP3/4 orthologue is not expressed during ANE restriction in the sea urchin embryo. Instead, our results indicate that ubiquitously expressed maternal sFRP-1 and Fzl1/2/7 signaling act together as early as the 32- to 60-cell stage to antagonize the ANE restriction mechanism mediated by Wnt/β-catenin and Wnt/JNK signaling. Then, starting from the blastula stage, Fzl5/8 signaling activates zygotic sFRP-1 within the ANE territory, where it works with the secreted Wnt antagonist Dkk1 (also activated by Fzl5/8 signaling) to antagonize Wnt1/Wnt8–Fzl5/8–JNK signaling in a negative feedback mechanism that defines the outer ANE territory boundary. Together, these data indicate that maternal and zygotic sFRP-1 protects the ANE territory by antagonizing the Wnt1/Wnt8–Fzl5/8–JNK signaling pathway throughout ANE restriction, providing precise spatiotemporal control of the mechanism responsible for the establishment of the ANE territory around the anterior pole of the sea urchin embryo.

Keywords

  • Developmental biology
  • Neuroectoderm patterning
  • Wnt signal transduction
  • Anterior–posterior
  • Deuterostome evolution
  • Gene regulatory networks
  • Dkk1
  • sFRP-1/2/5
  • Fzl1/2/7
  • Fzl5/8

Background

Metazoan embryos share a remarkably conserved toolkit of signal transduction pathways and transcription factors, which often are arranged into conserved gene regulatory networks (GRNs) that drive similar developmental processes. Conversely, these conserved toolkit components can also be re-arranged into novel GRNs that lead to morphological differences among species [1, 2]. While most evolutionary and developmental biology studies focus on these conserved toolkit genes, relatively few functional studies are performed on the novel genes that comprise a significant proportion of sequenced genomes [3, 4]. These novel genes can be a powerful mechanism for generating morphological diversity among animals, and most studies have been focused on this aspect [3, 5]. However, another important question that has been largely overlooked is what happens when novel gene products are incorporated into the more ancient signal transduction pathways and transcriptional regulatory networks that drive fundamental development processes and maintain adult tissue homeostasis in a variety of animals.

The molecular components involved in Wnt signaling are highly conserved in metazoans from cnidarians to humans. Three main branches have been identified: the “canonical” Wnt/β-catenin pathway and the “alternative” Wnt/JNK and Wnt/Ca2+ pathways. Each of these pathways uses a combination of secreted Wnt ligands and transmembrane Frizzled receptors as well as various co-receptors and secreted modulators to influence the activity of its respective intracellular signaling pathway. The specific developmental roles for Wnt signaling are also often remarkably conserved among many metazoan embryos. One of these is the gradient of Wnt signaling that is essential for territory patterning along the primary embryonic axis (anterior–posterior, oral–aboral, animal–vegetal). In most metazoans, high Wnt signaling specifies endoderm around the end of the primary axis where the blastopore will form, while low Wnt signaling levels allow for ectodermally derived sensory organ specification on the opposite side of the embryo [614]. In many deuterostome embryos (echinoderms, hemichordates, urochordates, cephalochordates, vertebrates), patterning along the primary anterior–posterior (AP) axis can be observed by the gradual restriction of the anterior neuroectoderm (ANE) gene regulatory network (GRN) activity to a region around the anterior pole of the embryo (for review see [28]). In deuterostome embryos in which AP neuroectoderm patterning has been studied, early ANE GRN members, such as Six3, initially are expressed broadly throughout the presumptive neuroectoderm territory [7, 1519]. Then, a mechanism that depends on the posterior-to-anterior gradient of Wnt/β-catenin signaling progressively eliminates ANE GRN expression from more posterior ectoderm, ultimately confining it to a territory around the anterior pole where secreted Wnt antagonists block Wnt signaling [7, 1923]. Once restricted around the anterior pole, these ANE territories subsequently give rise to structures ranging from the simple anterior sensory organs of invertebrate deuterostomes to the more complex vertebrate forebrain and eye fields [2429]. Importantly, comparative gene expression and functional studies among deuterostome embryos reveal significant similarities in the gene regulatory networks (GRNs) governing the specification and patterning of the territories from which anterior neurogenic organs arise [28], suggesting that they may be homologous.

Previous studies have shown that the ANE restriction mechanism in sea urchin embryos begins to downregulate ANE gene expression as early as the 32-cell stage when high Wnt/β-catenin signaling represses the expression of two early cardinal regulators of the ANE GRN, Six3 and FoxQ2, in the posterior half of the embryo, restricting their expression to the anterior hemisphere [19, 21]. In addition to antagonizing ANE GRN expression and activating endomesoderm specification, Wnt/β-catenin signaling also activates the expression of two secreted Wnt ligands, Wnt1 and Wnt8, in posterior endomesodermal blastomeres at the 32-cell stage. These ligands appear to diffuse to more anterior blastomeres, where they activate a Wnt/JNK signaling pathway through the Fzl5/8 receptor, which acts as a relay to further downregulate the expression of the ANE GRN in the ectoderm territory. Simultaneously, Fzl1/2/7–PKC signaling antagonizes Wnt/JNK signaling in ectodermal cells, preventing the elimination of ANE GRN expression from anterior-most cells during the initial and middle stages of ANE positioning. During the final phase of the process, Fzl5/8 signaling activates the expression of a secreted Wnt antagonist, Dkk1, in the cells around the anterior pole. Dkk1 prevents the downregulation of ANE factors within this territory by antagonizing Fzl5/8 signaling through a negative feedback mechanism [20], establishing a correctly sized ANE territory. As a result of this process, three early domains are established along the AP axis: endomesoderm around the posterior end; an equatorial ectodermal band that will form ventral and dorsal ectodermal structures separated by the ciliary band and associated nerves; and the anterior neuroectoderm domain around the anterior pole. These observations established that integrated information from all three of these Wnt signaling pathways patterns cell fates along the anterior–posterior axis in sea urchins, and we propose that these form a Wnt signaling network [20]. Remarkably, comparison of functional and expression studies among deuterostome embryos strongly suggests that aspects of this mechanism uncovered in the sea urchin embryo may be conserved among deuterostome embryos [28].

While much is known about many of the components of the individual signaling branches, relatively little is known about the specific molecular mechanisms that mediate coordinated interactions among them in any in vivo developmental model. Secreted extracellular Wnt modulators (e.g., sFRPs and Dkks) are obvious candidates for mediating these interactions during AP neuroectoderm patterning, since they have been shown to play essential roles during primary axis patterning in several metazoan embryos [20, 3032], including those of sea urchins and chordates. Phylogenetic analyses suggest that the eumetazoan ancestor possessed six Frizzled-related genes that included four Frizzled receptors (fzl1/2/7, fzl4, fzl5/8, fzl9/10) and two secreted Frizzled-related genes (sfrp-1/2/5 and sfrp3/4) [33, 34]. The sea urchin genome contains the full Frizzled-related complement, and all of these genes are expressed during early embryonic development except for sfrp3/4 [35, 36]. Because vertebrate sFRP3/4 orthologues (FrzBs) play critical roles in early AP patterning and anterior specification processes in vertebrates [3739], the silence of sfrp3/4 is curious. The core domain that each of these Frizzled-related genes contain is the Frizzled cysteine-rich domain (Fzl-CRD), which is critical for Wnt ligand interactions [40, 41]. Interestingly, the sea urchin also possesses a set of 15 novel Fzl-CRD-containing proteins of unknown function (see Additional file 1: Figure S1A) [34]. In 2002, Illies et al. [43] described the domain architecture and spatiotemporal expression of one of these novel Fzl-CRD-containing proteins; they termed secreted Frizzled-related protein 1 (sFRP-1) in early Strongylocentrotus purpuratus embryos that appears to be related to the ancient lineage of secreted Frizzled-related protein 3/4 (sFRP3/4) [35]. Similar to other sFRPs, this protein contains a signal sequence and at least one cysteine-rich domain (CRD), while lacking transmembrane domains. However, unlike sFRPs, this novel protein does not possess a Netrin domain [30, 42], but instead contains 4 tandem CRD domains with a single Ig domain situated in between CRD3 and CRD4 (see Fig. 1Aa). These four CRDs are well conserved with one another and with the CRDs of sFRPs and Frizzled receptors, maintaining the highly conserved spacing of the 10 characteristic cysteine residues. sfrp-1 is ubiquitously expressed during early blastula stages and then prominently expressed in both the endoderm and the ANE territory by mesenchyme blastula/early gastrula stages [43], overlapping spatiotemporally with the region in which the Wnt network is controlling the establishment ANE GRN around the anterior pole.

Here we present the first functional study of the novel secreted Frizzled-related protein 1 gene. Our data indicate that ubiquitously expressed, maternal sFRP-1 function is necessary, along with Fzl1/2/7 signaling, to antagonize the early ANE restriction mechanism mediated by Wnt/β-catenin and Wnt/JNK signaling. In addition, we found that Fzl5/8–JNK signaling activates zygotic expression of sFRP-1 in anterior cells during the later stages of ANE restriction, where sFRP-1 acts together with secreted Dkk1 to antagonize Fzl5/8–JNK signaling through a negative feedback mechanism to establish the ANE territory.

Results

sfrp-1 and sfrp3/4 expression during ANE restriction

The sea urchin genome contains at least 15 novel Fzl-CRD-containing genes [34, 44]. A phylogenetic analysis of the individual Fzl-CRD domains from these proteins indicates these proteins form six groups (Additional file 1: Figure S1A). In this study, we focus on a novel secreted Frizzled-related gene, termed sFRP-1 [43], that clusters with the Fzl-CRD domains of ancestral Frizzled receptors and sFRPs (Additional file 1: Figure S1A). Previously, Illies et al. [43] showed that sfrp-1 transcripts are expressed in a spatiotemporal profile consistent with a role in early AP patterning. Using northern blot and in situ hybridization approaches, they found that sfrp-1 transcripts were not expressed until early blastula stage. Using more sensitive qPCR analyses, we detected sfrp-1 transcripts in the fertilized egg and at the 60-cell stage (9 hpf) (see Fig. 5Ab). We were also able to detect ubiquitously expressed sfrp-1 transcripts by whole-mount in situ hybridization as early as the 60-cell stage (Fig. 1Aa). Consistent with the earlier report [43], high levels of sfrp-1 expression were detected during early to mid-blastula stages, when these transcripts were expressed broadly throughout the embryo (Fig. 1Ab, Ac). Subsequently, sfrp-1 expression was downregulated in the central ectoderm territory during mid-to-late blastula stages (Fig. 1Ad), resulting in localized expression in the ANE and posterior endomesoderm territories by the mesenchyme blastula/early gastrula stage (Fig. 1Ae). As a measure of ANE restriction, we assayed the downregulation of expression of the cardinal ANE regulatory factor foxq2 from lateral ectodermal cells, which initiates around 60-cell stage and terminates at mesenchyme blastula stage (24 hpf) (Fig. 1Af–j). These results indicate that sfrp-1 is expressed in all ectoderm cells in which ANE gene expression is downregulated by Wnt1/Wnt8–Fzl5/8–JNK signaling during the initial stages of ANE restriction. Then, sfrp-1 is restricted to the ANE territory around the same time that ANE restriction terminates [20]. In addition, the expression of sfrp-1 in the posterior endomesoderm cells during the mesenchyme blastula/early gastrula stage (Fig. 1Ae) suggests that sFRP-1 is also involved in the specification of this territory and/or the morphogenetic movements during gastrulation.
Fig. 1
Fig. 1

Spatiotemporal expression of sFRP-1 during ANE restriction. Aac sfrp-1 expression is first detected at the 32- to 60-cell stage and is present throughout the embryo until mid-blastula stage. Ad, Ae Between mesenchyme blastula stage and early gastrula, sfrp-1 is restricted to anterior and posterior blastomeres. Afj foxq2 expression is first detected at 32- to 60-cells stage in the anterior blastomeres and is progressively downregulated from posterior ectoderm cells from the 60-cell to mesenchyme blastula stages as previously shown [21]. Ako Diagram showing a model for the areas of Wnt/β-catenin, Fzl5/8–JNK, and Fzl1/2/7–PKC signaling during ANE restriction consistent with the data from [20]. Each individual diagram corresponds to the developmental stages depicted in the panels directly above. B Functional protein domain organization for the CRD containing proteins including sea urchin sFRP3/4 (a) and secreted Frizzled-related protein 1 (b). Scale bar = 20 μm

sFRP-1’s Fzl-CRD domains are related to those of sFRP3/4, suggesting that sFRP-1 may have emerged from the ancestral sFRP3/4 (Fig. 1B) [35]. Interestingly, tiling and transcriptome data suggest that the ancestral sea urchin sfrp3/4 gene is not transcribed during early sea urchin development [35]. To confirm these data, we performed qPCR analysis on embryos at several developmental time points during ANE restriction, which showed that only 1–4 sfrp3/4 transcripts per embryo were expressed at any developmental stage during ANE restriction (Additional file 1: Figure S1B), suggesting that in contrast to vertebrate embryos the ancestral sFRP3/4 is not necessary for early anterior–posterior development in sea urchin embryos.

sFRP-1 is necessary for ANE territory specification

The domain structure and spatial expression of sfrp-1 suggest that it could function to modulate Wnt signaling during ANE restriction. To test this hypothesis, we performed knockdowns with two different morpholino oligonucleotides and analyzed ANE GRN expression at mesenchyme blastula stage (24 hpf) (Fig. 2; Additional file 2: Figure S2). Whole-mount in situ hybridization (WMISH) showed that the cardinal ANE regulators six3 and foxq2, as well as downstream ANE GRN components dkk3, nkx3.2, sfrp-1/5 were downregulated in sFRP-1 morphants (Fig. 2A; Additional file 2: Fig. 2A). In addition, qPCR analysis showed that the expression of foxq2, nkx3.2, and dkk3 as well as that of two other components of the ANE GRN, hbn and zic2, was consistently downregulated in sFRP-1 morphants at the mesenchyme blastula stage (24 hpf) (Fig. 2B). These results show that sFRP-1 is necessary for the specification of the ANE territory, possibly through a role in antagonizing the ANE restriction mechanism mediated by Wnt/β-catenin and Wnt1/Wnt8/Fzl5/8–JNK signaling.
Fig. 2
Fig. 2

sFRP-1 is necessary for ANE specification. Aae six3, foxq2, dkk3, nkx3.2, and sfrp-1/5 expression in mesenchyme blastula stage control embryos (24 hpf). Agk Embryos injected with sFRP-1 morpholino 1 show complete elimination of ANE markers. B qPCR measurements from three different cultures of embryos showing the downregulation of ANE regulatory genes at mesenchyme blastula stage (24hpf) in sFRP-1 morphants. The y axis shows the fold change in gene expression for sFRP-1 morphants versus controls. Scale bar = 20 μm. MO, morpholino

sFRP-1 antagonizes Fzl5/8 signaling throughout ANE restriction

We previously identified two components (Dkk1 and Fzl1/2/7 signaling) of the molecular mechanism(s) necessary to antagonize Wnt1/Wnt8–Fzl5/8–JNK signaling emanating from posterior/vegetal blastomeres during ANE restriction. If each of these components is knocked down individually, Fzl5/8–JNK signaling appears to be upregulated, resulting in complete elimination of ANE GRN expression. Importantly, the expression of the ANE GRN can be rescued in Dkk1 and Fzl1/2/7 knockdown embryos if Fzl5/8 signaling is inhibited [20, 31]. Together, these results indicate that both Fzl1/2/7 signaling and Dkk1 are essential to establish the ANE territory. Based on the sFRP-1 morpholino knockdown phenotype, we reasoned that secreted sFRP-1 may also function to protect the ANE GRN by antagonizing Fzl5/8–JNK signaling. To begin to test this idea, we injected zygotes with synthetic sfrp-1 mRNA and found that expression of foxq2 expanded toward the posterior/vegetal pole at mesenchyme blastula stage (24 hpf) (Fig. 3A), suggesting that high levels of sFRP-1 interfere with Fzl5/8’s downregulation of the ANE GRN. Next, within each of the three batches of zygotes we injected one set with sFRP-1 MO1 and a second set with sFRP-1 MO1 and mRNA encoding a dominant-negative form of the Fzl5/8 receptor (ΔFzl5/8). As before, foxq2 expression was significantly downregulated or completely undetectable in embryos lacking sFRP-1 (Fig. 3Bb). In contrast, a large majority of fertilized embryos injected with sFRP-1 MO1 and ΔFzl5/8 mRNA showed expanded foxq2 expression (Fig. 3Bc), indicating that, in the absence of functional Fzl5/8, the ANE GRN is still activated in sFRP-1 morphants. Taken together, these results indicate that sFRP-1 is necessary to antagonize Fzl5/8–JNK signaling and therefore inhibit the downregulation of the ANE GRN (Fig. 3C).
Fig. 3
Fig. 3

Function of maternal and zygotic sFRP-1 during ANE restriction. A Compared to control embryos (a), embryos injected with sfrp-1 mRNA show expanded foxq2 expression (b). B In the absence of sFRP-1, foxq2 expression is completely eliminated from ANE territory (Bb), whereas sFRP-1 morphants co-injected with ΔFzl5/8 show expanded foxq2 expression (Bc). The number of embryos examined that show the representative phenotypes depicted is indicated in each panel. C A model diagram for ANE restriction during late blastula stages showing Wnt1/Wnt8–Fzl5/8–JNK signaling downregulates the transcription of fzl5/8 in posterior ectoderm, restricting its expression to the ANE territory. In the ANE, Fzl5/8 signaling activates dkk1 expression, antagonizing Wnt1/Wnt8–Fzl5/8–JNK signaling and establishing the ANE territory. Maternal and/or zygotic sFRP-1 is also necessary to antagonize Fzl5/8 signaling at this stage of development. The model is based data presented in this figure and from [20]. D Expression of foxq2 from 60-cell stage to mesenchyme blastula stage in control embryos (Dae), in translation-blocking sFRP-1 morphants (Dfj) and splice-blocking sFRP-1 morphants (Dko). MO, morpholino. Scale bar = 20 μm

The spatial and temporal expression patterns of sfrp-1 suggest it may function throughout the period of ANE restriction (32/60-cell stage to mesenchyme blastula). To test this hypothesis, we used separately a translation-blocking morpholino (sFRP-1 MO1) to knock down the function of both maternally and zygotically synthesized sFRP-1 mRNA and a splice-blocking morpholino (sFRP-1 MO2) to knock down only zygotic sFRP-1 activity and assayed for foxq2 expression. In translation-blocking morphants, foxq2 expression was completely downregulated in 60-cell stage embryos and downregulation was maintained until mesenchyme blastula stage (Fig. 3Df–j). In splice-blocking morphants, foxq2 expression was detected in 60-cell stage and 120-cell stage embryos (Fig. 3Dk, Dl) and then downregulated in early blastula stage and mesenchyme blastula stage embryos (Dm–o). Together, these results indicate that maternal and/or early zygotic sFRP-1 transcripts are necessary to antagonize Fzl5/8–JNK-mediated downregulation of ANE GRN from the beginning of the restriction process. Then, during the blastula stages, zygotic sFRP-1 activity is necessary to insulate the ANE territory by antagonizing Fzl5/8–JNK signaling.

sFRP-1 and Fzl1/2/7 signaling act together, but independently to antagonize ANE restriction

In a previous study, we showed that Fzl1/2/7–PKC signaling is necessary to antagonize the downregulation of the ANE GRN by Wnt/β-catenin and Fzl5/8–JNK signaling from as early as the 32- to 60-cell stage at the beginning of ANE restriction [20]. Above we showed that foxq2 expression was eliminated in sFRP-1 morphants during early cleavage stages (Fig. 3Df), mimicking the phenotype we observed when Fzl1/2/7–PKC signaling was blocked. Thus, it is possible that sFRP-1 plays a role either downstream of, or in parallel with, Fzl1/2/7 to antagonize the restriction process. To determine the relationship between sFRP-1 and Fzl1/2/7 signaling, we injected zygotes with Fzl1/2/7 morpholino oligonucleotides and observed expression of sfrp-1 in the embryos at multiple stages during ANE restriction. At the 60-cell stage, sfrp-1 was still expressed in the absence of Fzl1/2/7 signaling (cf. Figure 4Aa, Ad). However, starting from mid-blastula stage, sfrp-1 expression initially was lost in the whole embryo and the loss persisted in the anterior hemisphere throughout ANE restriction, although low levels of expression were reactivated in the posterior endomesoderm territory (Fig. 4Ae, Af). These data indicate that Fzl1/2/7 signaling is not necessary for sfrp-1 expression during early cleavage stages, but it might be necessary for its later zygotic expression in the anterior and posterior territories of the embryo. In the absence of Fzl1/2/7 signaling, Fzl5/8–JNK signaling is unchecked in the anterior half of the embryo; thus, Fzl5/8–JNK signaling in anterior blastomeres in the absence of Fzl1/2/7–PKC antagonism could alternatively be responsible for the downregulation of sfrp-1 in Fzl1/2/7 morphants. To distinguish between these alternatives, we compared sfrp-1 expression in embryos injected Fzl1/2/7 MO alone and those injected with Fzl1/2/7 MO and high levels of synthetic dkk1 mRNA (Fig. 4B). We have previously shown that Dkk1 acts as a secreted Wnt modulator that antagonizes the Wnt/JNK signaling-mediated downregulation of the ANE GRN [31]. sfrp-1 expression persisted in the embryos injected with Fzl1/2/7 MO along with dkk1 mRNA, while it was eliminated in the embryos injected with Fzl1/2/7 MO alone (Fig. 4Bb, Bc), indicating that in the absence of Fzl1/2/7 signaling, Fzl5/8 signaling downregulates sfrp-1 during the later stages of ANE restriction. Together, these observations indicate that maternal sFRP-1 works together with, but independently from, Fzl1/2/7–PKC signaling to antagonize Wnt/β-catenin and/or Wnt/JNK signaling that drive downregulation of the ANE GRN (Fig. 4C).
Fig. 4
Fig. 4

Control of sfrp-1 expression by the Wnt signaling network governing ANE restriction. A Fzl5/8–JNK signal-mediated downregulation of ANE gene expression is enhanced in the absence of Fzl1/2/7. Control embryos showing sfrp-1 expression at 60-cell (a), blastula (b) and mesenchyme blastula stage (c). Adf In Fzl1/2/7 MO injected embryos, sfrp-1 is expressed at the 60-cell stage (d), but downregulated in blastula (e) and mesenchyme blastula embryos (f). Bac sfrp-1 expression in Fzl1/2/7 morphants is rescued by overexpressing dkk1 mRNA. The number of embryos examined that show the representative phenotypes depicted is indicated in each panel. C A model diagram, showing that maternal sFRP-1 works together with, but independently from, Fzl1/2/7 signaling during the early stages of ANE restriction (Ca) and that zygotic sfrp-1 is part of the ANE GRN downregulated by Wnt/JNK signaling during later stages of the process (Cb). The model also shows that during later stages of ANE restriction the Fzl5/8 receptor is a member of the ANE GRN and Fzl5/8–JNK signaling downregulates fzl5/8 expression in the lateral ectoderm. The model is based on the data presented in this and the preceding figures, as well as data from [20]. MO, morpholino. Scale bar = 20 μm

sFRP-1 acts in parallel with Dkk1 downstream of Fzl5/8 signaling to establish the ANE territory

Fzl5/8 signaling activates a negative feedback loop by activating high levels of the secreted Wnt inhibitor Dkk1 around the anterior pole at the end of ANE restriction (late blastula [18 hpf]/mesenchyme blastula stages [24 hpf]). In our previous study, we showed that this high level of Dkk1 blocks Fzl5/8–JNK-mediated downregulation of the ANE GRN and establishes the perimeter of the ANE territory at this stage [20] (see Fig. 6). However, we did not investigate a potential involvement of Dkk1 during early stages of ANE restriction because dkk1 expression cannot be detected by WMISH until the end of the restriction process at mesenchyme blastula stage (Additional file 3: Figure S3). Low levels of dkk1 transcripts are detectable in zygotes and through mid-blastula stages by qPCR (Fig. 5Aa) which are similar to the expression levels of sfrp-1 during cleavage stages (Fig. 5b inset). Thus, we hypothesized that these levels of Dkk1 may be sufficient and necessary to antagonize Fzl5/8 signaling during early stages of ANE restriction (32- to 60-cell stage), along with early sFRP-1. To test this idea, we assayed for foxq2 expression in Dkk1 morphants and sFRP-1 morphants in the same batches of embryos at the very beginning of ANE restriction (late 32-cell stage; 7–8 hpf). As expected, foxq2 expression was severely downregulated in sFRP-1 knockdown embryos at the late 32-cell stage, but embryos injected with a previously characterized Dkk1 morpholino [20] showed no detectable difference in foxq2 expression when compared to control embryos (Fig. 5Ba–c). In both cases, foxq2 was completely eliminated in both sFRP-1 and Dkk1 knockdown embryos by the mesenchyme blastula/early gastrula stage (Fig. 5Bd–f). These results suggest that Dkk1 is only necessary during the later stages of ANE restriction.
Fig. 5
Fig. 5

sFRP-1 and Dkk1 antagonize Wnt signaling during final phase of ANE restriction. A qPCR measurements showing the temporal expression of dkk1 (a) and sfrp-1 (b) transcripts per embryo from egg to mesenchyme blastula stage of development. The inset in b shows the number of sfrp-1 transcripts per embryo in fertilized eggs and 60-cell embryos. B Comparing foxq2 expression between Dkk1 morphants (Bb, Be) and sFRP-1 morphants (Bc, Bf) during early and late stages of the ANE restriction. C Beginning at blastula stages, sfrp-1 is downregulated in embryos in the absence of functional Fzl5/8 signaling (eh). D A model diagram, showing that both zygotic sfrp-1 and dkk1 are activated by Fzl5/8 signaling in the ANE and that they work together in a negative feedback loop to antagonize Wnt1/Wnt8–Fzl5/8 signaling in the ANE territory. The model is based on the data presented in this and the preceding figures, as well as data from [20]. FE, fertilized egg; EB, early blastula; B, blastula; MB, mesenchyme blastula. MO, morpholino. Scale bar = 20 μm

The expression pattern of sfrp-1 appears to overlap those of fzl5/8 and dkk1 (cf. Additional file 1: Figure S3Ae, Ba, and Bb); thus, we hypothesized that Fzl5/8 signaling activates sfrp-1 in the ANE territory in addition to dkk1. To test this hypothesis, we injected zygotes with ΔFzl5/8 mRNA and assayed the expression of sfrp-1 in the embryos at multiple stages during ANE restriction. There was no difference in expression of sfrp-1 between control embryos and ΔFzl5/8 mRNA-injected embryos between the 60-cell and 120-cell stages (Fig. 5Ca, Cb, Ce, Cf). In contrast, expression of sfrp-1 was downregulated in ~ 45% of ΔFzl5/8 mRNA-injected embryos at the hatched blastula stage (16 hpf) (n = 73/162) and the percentage of embryos lacking detectable sfrp-1 increased to ~ 94% at the mesenchyme blastula stage (24 hpf) (n = 181/193) (Fig. 5Cg, Ch). Taken together, these results suggest that Fzl5/8 signaling is required to activate zygotic sfrp-1 expression beginning midway through ANE restriction, where it acts in parallel with Dkk1 in a negative feedback mechanism to antagonize Fzl5/8 signaling around the anterior pole (Fig. 5D).

Discussion

We present the first functional characterization of the novel secreted Frizzled-related 1 (sFRP-1) protein, which is expressed during early anterior–posterior neuroectoderm specification and patterning in the sea urchin embryo. Our analyses indicate that maternally supplied sFRP-1 works in concert with, but independently from, the Fzl1/2/7 signaling pathway to antagonize the downregulation of ANE GRN expression by Fzl5/8–JNK signaling during the early stages of ANE restriction (60-cell to blastula stages). Then, Fzl5/8 signaling activates zygotic sFRP-1 around the anterior pole where it works in parallel with Dkk1 in a negative feedback signaling mechanism to antagonize Fzl5/8–JNK signaling during the final phase of ANE restriction, establishing the outer boundary of the ANE territory. Interestingly, sFRP-1 is similar to several poorly characterized genes in many metazoan species that contain one or more well-conserved Wnt binding Fzl-CRD domains [34]. Our study strongly suggests that these Fzl-CRD-containing proteins may be important and possibly novel components of the Wnt signaling mechanisms in the species in which they exist.

We previously showed that there are at least two critical interactions among the Wnt signaling branches during ANE restriction as early as the 32- to 60-cell stages in sea urchin embryos. At this time, Wnt/β-catenin signaling in posterior blastomeres activates the expression of Wnt1 and Wnt8. Our expression and functional data [20] suggest that these ligands diffuse into more anterior ectodermal blastomeres where they activate Fzl5/8–JNK signaling [20], acting as a relay mechanism between Wnt/β-catenin in posterior endomesodermal cells and Wnt/JNK signaling in anterior ectodermal cells (Fig. 6). At the same time, Fzl1/2/7 signaling antagonizes both Wnt/β-catenin and Fzl5/8–JNK signaling, preventing these pathways from being upregulated and completely eliminating the ANE GRN as early as the 32- to 60-cell stage [20]. Here, our data strongly suggest that sFRP-1 activity is necessary from the very beginning to antagonize the activity of Fzl5/8–JNK signaling only in the anterior half of the embryo (Fig. 3). The results from these experiments parallel those used to determine the function of Fzl1/2/7 signaling [20], indicating that both maternally supplied mechanisms are critical to moderate Fzl5/8–JNK signaling from the beginning of the restriction process. To date, the exact molecular mechanism(s) by which Fzl1/2/7–PKC signaling antagonizes Fzl5/8–JNK signaling during the early stages of ANE restriction are unknown. It is possible that Fzl1/2/7 signaling antagonizes Fzl5/8–JNK signaling at the intracellular and/or transcriptional level. Alternatively, Fzl1/2/7 signaling could activate a secreted modulator like sFRP-1 that blocks Wnt1/Wnt8–Fzl5/8–JNK signaling at the extracellular level. Our data show that Fzl5/8–JNK signaling activates zygotic sfrp-1, not Fzl1/2/7 signaling, indicating that sFRP-1 is not a secreted factor activated downstream of Fzl1/2/7 signaling. Instead, we propose that maternally supplied secreted sFRP-1 interferes with Wnt1 and Wnt8 in the extracellular space, preventing the activation of Fzl5/8–JNK signaling in anterior blastomeres together with, but independent from, Fzl1/2/7 signaling during the early stages of the ANE restriction mechanism.
Fig. 6
Fig. 6

A new model for the Wnt signaling network governing ANE restriction in the sea urchin embryo and the evolution of sFRP3/4 and sFRP-1 in deuterostomes. Aa Early downregulation of the ANE GRN from posterior blastomeres. (Posterior half of the embryo) A broad, maternal regulatory mechanism is able to activate the ANE GRN throughout the embryo by the 32-cell stage, but nβ-catenin signaling prevents the expression of the ANE GRN in the posterior half of the 32-cell embryo through an unknown mechanism and activates Wnt1 and Wnt8 expression at the 32-cell stage. In addition, around the 32- to 60-cell stage sFRP-1 and Fzl1/2/7 signaling antagonize the downregulation of the ANE GRN in the anterior hemisphere [20]. Ab Downregulation of the ANE GRN from cells in the lateral ectoderm domain and the establishment of the ANE around the anterior pole. (Anterior half of the embryo) Around the 32- to 60-cell stage (7–9 hpf), secreted Wnt1 and Wnt8 diffuse into more anterior ectodermal blastomeres (Wnt8 expression is activated throughout the equitorial ectoderm territory) and signal through the Fzl5/8 receptor, activating the JNK pathway. This Wnt/JNK pathway progressively downregulates ANE GRN expression from the central ectodermal territory during the early to late blastula stages (12–18 hpf). Within the same ectodermal cells, sFRP-1 and Fzl1/2/7 signaling antagonize Wnt1/Wnt8–Fzl5/8-JNK-mediated downregulation of the ANE GRN. Around the mid-blastula stage (16 hpf), an anterior signaling center activated by the cardinal ANE transcriptional regulator FoxQ2 secretes the Wnt modulators Dkk3 and sFRP-1/5 within the regressing ANE territory. Dkk3 and low levels of sFRP-1/5 are necessary to stimulate the Fzl5/8–JNK signaling during the later stages of ANE restriction. During the final phase of the process from early to late blastula stages (18–24 hpf), Fzl5/8 signaling activates the expression of the secreted Wnt antagonists sFRP-1 and Dkk1 in the anterior-most cells around the anterior pole. These antagonists establish a correctly sized ANE territory by preventing the downregulation of ANE factors by antagonizing Fzl5/8 signaling through a negative feedback mechanism [20]. B Schematic representation of the expansion of sFRP3/4 paralogues and sFRP-1 during deuterostome evolution

Our data also show that Wnt1/Wnt8–Fzl5/8–JNK signaling must be limited throughout ANE restriction to maintain the steady posterior-to-anterior downregulation of ANE GRN members between the 60-cell and mesenchyme blastula stages [20] (Fig. 6Aa). In previous studies, we have shown that different molecular mechanisms activate two secreted anterior Wnt modulators, sFRP-1/5 and Dkk1 (FoxQ2 activates sfrp-1/5 and Fzl5/8 signaling activates dkk1). Both of these modulators must antagonize Fzl5/8 signaling in anterior ectoderm to maintain the correct rate of ANE GRN downregulation and the establishment of the final ANE territory beginning around the middle of the restriction process (mid-blastula stage) [20, 31]. Here, we show that zygotic sfrp-1 expression is activated by Fzl5/8 signaling around the same time as zygotic dkk1 and sfrp-1/5. Importantly, we show that zygotic sFRP-1 activity is necessary starting around mid-blastula stages to antagonize ANE restriction. Thus, it appears that the negative feedback mechanism activated by Fzl5/8 signaling during these stages activates two secreted Wnt modulators, sFRP-1 and Dkk1, that act in parallel, along with sFRP-1/5, to block Fzl5/8 signaling around the anterior pole and establish the final ANE territory (Fig. 6Ab pathway in red). Interestingly, both of these secreted modulators are essential to prevent downregulation of the ANE GRN because knocking down either one individually allows ANE downregulation to continue to the anterior pole. Together, these data are consistent with the idea that the early role of both maternal sFRP-1 and Fzl1/2/7 signaling is to separately act to moderate the activity of Fzl5/8–JNK signaling so that the wave of posterior-to-anterior downregulation of ANE GRN expression occurs at a specific rate. Then, in a coordinated spatiotemporal transition during the middle of ANE restriction, the cardinal transcriptional regulator FoxQ2 and Fzl5/8 signaling turn on the zygotic expression of three secreted Wnt modulators whose separate, but combined activity, in addition to the possible negative input of Fzl1/2/7 signaling, is able to build to a level that is capable of stopping the ANE restriction mechanism and defining the outer boundary of the ANE territory.

The eumetazoan ancestor appears to have possessed a set of Frizzled-CRD containing genes including four receptors (Fzl1/2/7, Fzl5/8, Fzl9/10, and Fzl4) and two secreted Wnt signaling modulators (sFRP-1/2/5 and sFRP3/4). This core ancestral gene group is thought to have been maintained in many invertebrate metazoan species until whole genome duplications increased the number of orthologues in vertebrates [33, 34]. The unique domain architecture of protein families has traditionally been considered to be a result of duplication and modifications from a common ancestral gene [45]. Consistent with this idea, the vertebrate sFRP3/4s, urochordate sFRP3/4a and b, and the sea urchin sFRP3/4 maintained the domain organization of the original/ancestral sFRP3/4. sFRP-1 appears to be related to ancestral sFRP3/4 s [35]; however, the domain organization of sFRP-1 is novel, containing 4 tandemly arrayed Fzl-CRD domains and an Ig domain instead of one Fzl-CRD and Netrin domain. Interestingly, recent phylogenetic studies indicate that it is not uncommon for several novel Fzl-CRD-containing genes to exist in various taxa in addition to the more conserved core group of Fzl-CRD containing genes [46, 47]. Similar to the domain structure of sFRP-1, many of the novel proteins encoded by these genes are predicted to be secreted and they often contain one or more Fzl-CRD domains related to the Frizzled receptors or sFRPs [34, 48]. These data and others led Pei and Grishin to propose that Fzl-CRD domains may act as “mobile evolutionary units” that undergo domain fusion events, bringing new genes into Wnt signaling in the species in which they exist [48]. Given the unique domain architecture of sea urchin sFRP-1, it is thus possible that one or more of these mobile Fzl-CRD evolutionary units may have been involved in a domain fusion event(s) that lead to a novel gene related to the ancestral sFRP3/4 (Fig. 6B). Interestingly, the echinoderm sea star genome contains at least four genes that are related to sFRP-1 and possess a similar domain architecture (Fig. 6B), whereas hemichordates, which from a sister phylum with echinoderms, appear to lack any such gene. Together, these data suggest that sFRP-1 may have emerged after the divergence of echinoderms and hemichordates and then become integrated into the Wnt signaling network governing AP patterning in the sea urchin embryo.

Several possible outcomes can arise once a new functional gene appears in a genome. For example, if the new gene emerges from a duplication, it could play redundant functions as the paralogue, leading to new morphologies if spatiotemporal expression is different from the original gene.

The new gene could also take over the role of the ancestral gene, allowing the ancestral gene to take on a new role in a different territory and/or at different developmental stages [1, 5, 49]. We find it interesting that the ancestral sea urchin sfrp3/4 gene is not expressed during early embryonic AP specification and patterning given the prominent role the sFRP3/4 orthologue FrzB plays during AP neuroectoderm patterning in vertebrate deuterostomes. In Xenopus and zebrafish embryos, FrzB is expressed in the ANE territory (anterior pre-chordal plate) where it is necessary to antagonize posterior-to-anterior Wnt signaling and help establish the territory that will form the forebrain and eye field [3739]. While there are no functional studies on sFRP3/4 outside of the vertebrates, sfrp3/4 is expressed in anterior regions of hemichordate embryos during gastrula stages, as in vertebrates (Chris Lowe and Sebastien Darras labs, personal communication), suggesting that this ancestral sFRP3/4 may play a role in early AP neuroectoderm patterning in these organisms. Thus, it is tempting to speculate that sFRP-1 may have assumed the ancestral role of sFRP3/4 in the sea urchin embryo and that other deuterostome embryos may have retained it.

Conclusion

We have a limited understanding of how the different Wnt signaling branches involved in Wnt networks interact at the extracellular, the intracellular, or transcriptional levels to control one another’s activity in an in vivo developmental context. In this study, we have shown that the novel sea urchin protein, sFRP-1, is a critical member of a growing list of extracellular Wnt modulators, including Dkk1, Dkk3, and sFRP-1/5, that precisely control how information from the Wnt/β-catenin, Wnt/JNK, and Wnt/Ca2 + pathways is integrated during specification and patterning of territories along the AP axis in sea urchin embryos. Given the relative lack of attention paid to the functional role of novel genes in development, our results also provide an important illustration of how these genes can become key players in the otherwise highly conserved signaling pathways that govern fundamental developmental mechanisms.

Methods

Embryo cultures

Strongylocentrotus purpuratus were obtained from Monterey Abalone Company, Monterey, CA, and Point Loma Marine Invertebrate Lab, Lakeside, CA. The adult sea urchins were injected with 0.5 M KCL into their body cavities in order to collect the eggs and sperm. The eggs were washed two times with artificial sea water (ASW) and then fertilized in a glass beaker or a plastic culture dish by adding a 1:1000 dilution of sperm. Once fertilized, embryos were cultured in artificial seawater (ASW) at 15 °C.

mRNA and morpholino injections

Double-stranded DNA was synthesized (Integrated DNA Technologies) based on the published full-length sequence [43] and the sea urchin genome sequence [44]. The full-length sfrp-1 clone was inserted into pCS2 + vector using the following primers: Forward 5′-GCGATGGAGTTTCCACCTCA-3′; Reverse 5′-GAAGACTCACACAGCTCCCG-3′. sFRP-l-pCS2 was linearized with NotI, and mRNA was synthesized using the Sp6 mMessage mMachine Kit (Ambion). Overexpression studies were performed by injecting ~ 20 pL of full-length sfrp-1 (2–3 μg/μL) and dkk1 (3 μg/μL) as well as ΔFzl5/8 (2.0 μg/μL) mRNA into zygotes.

For loss-of-function experiments, two different morpholino-substituted oligonucleotides were designed from S. purpuratus EST and genomic sequences [43]. A splice-blocking morpholino was designed to target the first exon–intron boundary of sfrp-1, resulting in a transcript lacking sequence from the second exon. The morpholinos were produced by Gene Tools LLC (Eugene, OR). The sequences and injection concentrations were as follows: sFRP-1 MO1 (translation blocking): 5′-CGCTGTGACAGGTGTTCTCTTCGAT-3′ (0.75–0.85 mM); sFRP-1 MO2 (splice blocking): 5′-CGGAAGATATTATAGGCATACCTGT-3′ (2.25–2.5 mM); Dkk1 MO1: 5′-GCGTCTAAATCCTAAATTCCTTCCT-3′ (1.5–1.6 mM) [20].

For microinjections, eggs were de-jellied by passing them through 74 μm mesh Nitex. The eggs were arrayed in rows on a plastic culture dish coated with 25% protamine sulfate and fertilized by addition of diluted sperm. Immediately after fertilization, embryos were injected with a solution containing 15% FITC (2.5 μg/mL), 20% glycerol, and morpholino oligonucleotides and embryos were cultured at 15° C. Microinjection experiments were performed using at least three different batches of embryos, consisting of 30–200 embryos in each experiment. Experiments were considered conclusive only if a change in phenotype or marker expression was observed in at least 85% of the injected embryos.

Whole-mount in situ hybridization

Probes for each gene analyzed correspond to the full-length cDNA sequence. In situ hybridization and detection by alkaline phosphatase staining were carried out as previously described [19, 20, 50].

Quantitative polymerase chain reaction (qPCR)

qPCR experiments were performed as described previously [19]. For each experiment, embryos from three different mating pairs were used and each reaction was carried out in triplicate. The primers used for qPCR reaction were: sFRP-1, Forward-5′CGAGACGACTATTGCAGATG3′; Reverse- 5′ATTCCTCAGGGGAGTTAGG3′ and Dkk1, Forward-5′GTGTTCGCAAGGTCTCTC3′ and Reverse-5′GTCGTTCTTGCTCGGAAG3′. Primer set information for the rest of the ANE GRN genes is provided in [20]. ΔCt was used to calculate expression level for sfrp-1 relative to z12 in real-time quantitative PCR experiments. To determine the expression levels, the numbers of transcripts per embryo were estimated based on the ΔCt value of z12 transcript [51]. In differential expression comparisons between control and perturbed embryos mitochondrial 12 s RNA Ct values were used to normalize the relative concentration of mRNA; a twofold or higher change in gene expression level was considered to be significant.

Phylogenetic analysis

For the phylogenetic analysis, we used truncated amino acid sequences of the Fzl-CRD domains from each protein (Additional file 4: Table S1). The extracted sequences were aligned using Muscle [52] and manually edited with BioEdit [53]. Phylogenetic relationships among them were estimated using maximum likelihood and Bayesian approaches. We run maximum likelihood analyses in IQ-Tree ver 1.5.5 [54] as implemented in the IQ-Tree web server [55] last accessed on June 2017 and evaluated support for the nodes with the ultrafast bootstrap method [56]. We run Bayesian analyses in MrBayes version 3.2 [57], setting four simultaneous chains for 2 × 107 generations, sampling trees every 1000 generations, and using default priors. We assessed convergence by measuring the standard deviation of the split frequency among parallel chains. We summarized results with a majority-rule consensus of trees collected after convergence was reached.

Declarations

Authors’ contributions

AK, MM, SD, and RCR planned, performed, and analyzed experiments. AK and RCR prepared the manuscript. All authors read and approved the final manuscript.

Acknowledgements

We thank Dr. Robert Angerer for his careful reading and editing of the manuscript and Dr. Federico Hoffman for his assistance with the phylogenetic analysis. Support for this project was provided to RCR by NIH R15HD088272-01 as well as the Office of Research and Development, and Department of Biological Sciences at Mississippi State University.

Competing interests

The authors declare that they have no competing interests.

Availability of data and materials

The datasets used and/or analyzed during the current study are available from the corresponding author on reasonable request.

Consent for publication

Not applicable.

Ethics approval and consent to participate

Not applicable.

Publisher’s Note

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Open AccessThis article is distributed under the terms of the Creative Commons Attribution 4.0 International License (http://creativecommons.org/licenses/by/4.0/), which permits unrestricted use, distribution, and reproduction in any medium, provided 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 Creative Commons Public Domain Dedication waiver (http://creativecommons.org/publicdomain/zero/1.0/) applies to the data made available in this article, unless otherwise stated.

Authors’ Affiliations

(1)
Department of Biological Sciences, Mississippi State University, Mississippi State, MS 39762, USA
(2)
School of Pharmacy, University of Mississippi, Oxford, MS, USA

References

  1. Prud’homme B, Gompel N, Carroll SB. Emerging principles of regulatory evolution. Proc Natl Acad Sci USA. 2007;104(Suppl 1):8605–12.View ArticlePubMedPubMed CentralGoogle Scholar
  2. Peter IS, Davidson EH. Implications of developmental gene regulatory networks inside and outside developmental biology. Curr Top Dev Biol. 2016;117:237–51.View ArticlePubMedGoogle Scholar
  3. Khalturin K, Hemmrich G, Fraune S, Augustin R, Bosch TC. More than just orphans: are taxonomically-restricted genes important in evolution? Trends Genet. 2009;25(9):404–13.View ArticlePubMedGoogle Scholar
  4. Foret S, Knack B, Houliston E, Momose T, Manuel M, Queinnec E, Hayward DC, Ball EE, Miller DJ. New tricks with old genes: the genetic bases of novel cnidarian traits. Trends Genet. 2010;26(4):154–8.View ArticlePubMedGoogle Scholar
  5. Neme R, Tautz D. Phylogenetic patterns of emergence of new genes support a model of frequent de novo evolution. BMC Genom. 2013;14:117.View ArticleGoogle Scholar
  6. Adamska M, Degnan SM, Green KM, Adamski M, Craigie A, Larroux C, Degnan BM. Wnt and TGF-β expression in the sponge Amphimedon queenslandica and the origin of metazoan embryonic patterning. PLoS ONE. 2007;2(10):e1031.View ArticlePubMedPubMed CentralGoogle Scholar
  7. Darras S, Gerhart J, Terasaki M, Kirschner M, Lowe CJ. β-Catenin specifies the endomesoderm and defines the posterior organizer of the hemichordate Saccoglossus kowalevskii. Development. 2011;138(5):959–70.View ArticlePubMedPubMed CentralGoogle Scholar
  8. Momose T, Derelle R, Houliston E. A maternally localised Wnt ligand required for axial patterning in the cnidarian Clytia hemisphaerica. Development. 2008;135(12):2105–13.View ArticlePubMedGoogle Scholar
  9. Logan CY, Miller JR, Ferkowicz MJ, McClay DR. Nuclear β-catenin is required to specify vegetal cell fates in the sea urchin embryo. Development. 1999;126(2):345–57.PubMedGoogle Scholar
  10. Wikramanayake AH, Hong M, Lee PN, Pang K, Byrum CA, Bince JM, Xu R, Martindale MQ. An ancient role for nuclear β-catenin in the evolution of axial polarity and germ layer segregation. Nature. 2003;426(6965):446–50.View ArticlePubMedGoogle Scholar
  11. Henry JQ, Perry KJ, Martindale MQ. β-Catenin and early development in the gastropod, Crepidula fornicata. Integr Comp Biol. 2010;50:icq076.Google Scholar
  12. Henry JQ, Perry KJ, Wever J, Seaver E, Martindale MQ. β-catenin is required for the establishment of vegetal embryonic fates in the nemertean, Cerebratulus lacteus. Dev Biol. 2008;317(1):368–79.View ArticlePubMedGoogle Scholar
  13. Niehrs C. On growth and form: a Cartesian coordinate system of Wnt and BMP signaling specifies bilaterian body axes. Development. 2010;137(6):845–57.View ArticlePubMedGoogle Scholar
  14. Petersen CP, Reddien PW. Wnt signaling and the polarity of the primary body axis. Cell. 2009;139(6):1056–68.View ArticlePubMedGoogle Scholar
  15. Steinmetz PR, Urbach R, Posnien N, Eriksson J, Kostyuchenko RP, Brena C, Guy K, Akam M, Bucher G, Arendt D. Six3 demarcates the anterior-most developing brain region in bilaterian animals. EvoDevo. 2010;1(1):1.View ArticleGoogle Scholar
  16. Kozmik Z, Holland ND, Kreslova J, Oliveri D, Schubert M, Jonasova K, Holland LZ, Pestarino M, Benes V, Candiani S. Pax-Six-Eya-Dach network during amphioxus development: conservation in vitro but context specificity in vivo. Dev Biol. 2007;306(1):143–59.View ArticlePubMedGoogle Scholar
  17. Lagutin OV, Zhu CC, Kobayashi D, Topczewski J, Shimamura K, Puelles L, Russell HR, McKinnon PJ, Solnica-Krezel L, Oliver G. Six3 repression of Wnt signaling in the anterior neuroectoderm is essential for vertebrate forebrain development. Genes Dev. 2003;17(3):368–79.View ArticlePubMedPubMed CentralGoogle Scholar
  18. Posnien N, Koniszewski ND, Hein HJ, Bucher G. Candidate gene screen in the red flour beetle Tribolium reveals six3 as ancient regulator of anterior median head and central complex development. PLoS Genet. 2011;7(12):e1002416.View ArticlePubMedPubMed CentralGoogle Scholar
  19. Wei Z, Yaguchi J, Yaguchi S, Angerer RC, Angerer LM. The sea urchin animal pole domain is a Six3-dependent neurogenic patterning center. Development. 2009;136(7):1179–89.View ArticlePubMedPubMed CentralGoogle Scholar
  20. Range RC, Angerer RC, Angerer LM. Integration of canonical and noncanonical Wnt signaling pathways patterns the neuroectoderm along the anterior–posterior axis of sea urchin embryos. PLoS Biol. 2013;11(1):e1001467.View ArticlePubMedPubMed CentralGoogle Scholar
  21. Yaguchi S, Yaguchi J, Angerer RC, Angerer LM. A Wnt-FoxQ2-nodal pathway links primary and secondary axis specification in sea urchin embryos. Dev Cell. 2008;14(1):97–107.View ArticlePubMedGoogle Scholar
  22. Kiecker C, Niehrs C. A morphogen gradient of Wnt/β-catenin signalling regulates anteroposterior neural patterning in Xenopus. Development. 2001;128(21):4189–201.PubMedGoogle Scholar
  23. Nordstrom U, Jessell TM, Edlund T. Progressive induction of caudal neural character by graded Wnt signaling. Nat Neurosci. 2002;5(6):525–32.View ArticlePubMedGoogle Scholar
  24. Burke RD, Moller DJ, Krupke OA, Taylor VJ. Sea urchin neural development and the metazoan paradigm of neurogenesis. Genesis. 2014;52(3):208–21.View ArticlePubMedGoogle Scholar
  25. Castro A, Becerra M, Manso MJ, Anadón R. Neuronal organization of the brain in the adult amphioxus (Branchiostoma lanceolatum): a study with acetylated tubulin immunohistochemistry. J Comp Neurol. 2015;523(15):2211–32.View ArticlePubMedGoogle Scholar
  26. Cavodeassi F. Integration of anterior neural plate patterning and morphogenesis by the Wnt signaling pathway. Dev Neurobiol. 2014;74(8):759–71.View ArticlePubMedGoogle Scholar
  27. Pani AM, Mullarkey EE, Aronowicz J, Assimacopoulos S, Grove EA, Lowe CJ. Ancient deuterostome origins of vertebrate brain signalling centres. Nature. 2012;483(7389):289–94.View ArticlePubMedPubMed CentralGoogle Scholar
  28. Range R. Specification and positioning of the anterior neuroectoderm in deuterostome embryos. Genesis. 2014;52(3):222–34.View ArticlePubMedGoogle Scholar
  29. Garner S, Zysk I, Byrne G, Kramer M, Moller D, Taylor V, Burke RD. Neurogenesis in sea urchin embryos and the diversity of deuterostome neurogenic mechanisms. Development. 2016;143(2):286–97.View ArticlePubMedGoogle Scholar
  30. Bovolenta P, Esteve P, Ruiz JM, Cisneros E, Lopez-Rios J. Beyond Wnt inhibition: new functions of secreted Frizzled-related proteins in development and disease. J Cell Sci. 2008;121(Pt 6):737–46.View ArticlePubMedGoogle Scholar
  31. Range RC, Wei Z. An anterior signaling center patterns and sizes the anterior neuroectoderm of the sea urchin embryo. Development. 2016;143(9):1523–33.View ArticlePubMedPubMed CentralGoogle Scholar
  32. Niehrs C. Function and biological roles of the Dickkopf family of Wnt modulators. Oncogene. 2006;25(57):7469–81.View ArticlePubMedGoogle Scholar
  33. Lee PN, Pang K, Matus DQ, Martindale MQ. A WNT of things to come: evolution of Wnt signaling and polarity in cnidarians. Semin Cell Dev Biol. 2006;17(2):157–67.View ArticlePubMedGoogle Scholar
  34. Yan J, Jia H, Ma Z, Ye H, Zhou M, Su L, Liu J, Guo AY. The evolutionary analysis reveals domain fusion of proteins with Frizzled-like CRD domain. Gene. 2014;533(1):229–39.View ArticlePubMedGoogle Scholar
  35. Croce JC, Wu SY, Byrum C, Xu R, Duloquin L, Wikramanayake AH, Gache C, McClay DR. A genome-wide survey of the evolutionarily conserved Wnt pathways in the sea urchin Strongylocentrotus purpuratus. Dev Biol. 2006;300(1):121–31.View ArticlePubMedPubMed CentralGoogle Scholar
  36. Robert N, Lhomond G, Schubert M, Croce JC. A comprehensive survey of Wnt and frizzled expression in the sea urchin Paracentrotus lividus. Genesis. 2014;52(3):235–50.View ArticlePubMedGoogle Scholar
  37. Leyns L, Bouwmeester T, Kim SH, Piccolo S, De Robertis EM. Frzb-1 is a secreted antagonist of Wnt signaling expressed in the Spemann organizer. Cell. 1997;88(6):747–56.View ArticlePubMedPubMed CentralGoogle Scholar
  38. Wang S, Krinks M, Lin K, Luyten FP, Moos M Jr. Frzb, a secreted protein expressed in the Spemann organizer, binds and inhibits Wnt-8. Cell. 1997;88(6):757–66.View ArticlePubMedGoogle Scholar
  39. Lu FI, Thisse C, Thisse B. Identification and mechanism of regulation of the zebrafish dorsal determinant. Proc Natl Acad Sci USA. 2011;108(38):15876–80.View ArticlePubMedPubMed CentralGoogle Scholar
  40. Bafico A, Gazit A, Pramila T, Finch PW, Yaniv A, Aaronson SA. Interaction of frizzled related protein (FRP) with Wnt ligands and the frizzled receptor suggests alternative mechanisms for FRP inhibition of Wnt signaling. J Biol Chem. 1999;274(23):16180–7.View ArticlePubMedGoogle Scholar
  41. Oishi I, Suzuki H, Onishi N, Takada R, Kani S, Ohkawara B, Koshida I, Suzuki K, Yamada G, Schwabe GC, et al. The receptor tyrosine kinase Ror2 is involved in non-canonical Wnt5a/JNK signalling pathway. Genes Cells Devot Mol Cell Mech. 2003;8(7):645–54.View ArticleGoogle Scholar
  42. Chong JM, Uren A, Rubin JS, Speicher DW. Disulfide bond assignments of secreted Frizzled-related protein-1 provide insights about Frizzled homology and netrin modules. J Biol Chem. 2002;277(7):5134–44.View ArticlePubMedGoogle Scholar
  43. Illies MR, Peeler MT, Dechtiaruk A, Ettensohn CA. Cloning and developmental expression of a novel, secreted frizzled-related protein from the sea urchin, Strongylocentrotus purpuratus. Mech Dev. 2002;113(1):61–4.View ArticlePubMedGoogle Scholar
  44. Sea Urchin Genome Sequencing C, Sodergren E, Weinstock GM, Davidson EH, Cameron RA, Gibbs RA, Angerer RC, Angerer LM, Arnone MI, Burgess DR, et al. The genome of the sea urchin Strongylocentrotus purpuratus. Science. 2006;314(5801):941–52.View ArticleGoogle Scholar
  45. Vogel C, Teichmann SA, Pereira-Leal J. The relationship between domain duplication and recombination. J Mol Biol. 2005;346(1):355–65.View ArticlePubMedGoogle Scholar
  46. Minami Y, Oishi I, Endo M, Nishita M. Ror-family receptor tyrosine kinases in noncanonical Wnt signaling: their implications in developmental morphogenesis and human diseases. Dev Dyn. 2010;239(1):1–15.PubMedGoogle Scholar
  47. Wang L, Shao YY, Ballock RT. Carboxypeptidase Z (CPZ) links thyroid hormone and Wnt signaling pathways in growth plate chondrocytes. J Bone Min Res. 2009;24(2):265–73.View ArticleGoogle Scholar
  48. Pei J, Grishin NV. Cysteine-rich domains related to Frizzled receptors and Hedgehog-interacting proteins. Protein Sci Publ Protein Soc. 2012;21(8):1172–84.View ArticleGoogle Scholar
  49. Cheatle Jarvela AM, Hinman VF. Evolution of transcription factor function as a mechanism for changing metazoan developmental gene regulatory networks. Evodevo. 2015;6(1):3.View ArticlePubMedPubMed CentralGoogle Scholar
  50. Sethi AJ, Wikramanayake RM, Angerer RC, Range RC, Angerer LM. Sequential signaling crosstalk regulates endomesoderm segregation in sea urchin embryos. Science. 2012;335(6068):590–3.View ArticlePubMedPubMed CentralGoogle Scholar
  51. Wang DG, Kirchhamer CV, Britten RJ, Davidson EH. SpZ12-1, a negative regulator required for spatial control of the territory-specific CyIIIa gene in the sea urchin embryo. Development. 1995;121(4):1111–22.PubMedGoogle Scholar
  52. Edgar RC. MUSCLE: a multiple sequence alignment method with reduced time and space complexity. BMC Bioinform. 2004;5:113.View ArticleGoogle Scholar
  53. Ta H. BioEdit: a user-friendly biological sequence alignment editor and analysis program for Windows 95/98/NT. Nucl Acids Symp Ser. 1999;41:95–8.Google Scholar
  54. Nguyen LT, Schmidt HA, von Haeseler A, Minh BQ. IQ-TREE: a fast and effective stochastic algorithm for estimating maximum-likelihood phylogenies. Mol Biol Evol. 2015;32(1):268–74.View ArticlePubMedGoogle Scholar
  55. Trifinopoulos J, Nguyen LT, von Haeseler A, Minh BQ. W-IQ-TREE: a fast online phylogenetic tool for maximum likelihood analysis. Nucl Acids Res. 2016;44(W1):W232–5.View ArticlePubMedPubMed CentralGoogle Scholar
  56. Minh BQ, Nguyen MA, von Haeseler A. Ultrafast approximation for phylogenetic bootstrap. Mol Biol Evol. 2013;30(5):1188–95.View ArticlePubMedPubMed CentralGoogle Scholar
  57. Ronquist F, Teslenko M, van der Mark P, Ayres DL, Darling A, Hohna S, Larget B, Liu L, Suchard MA, Huelsenbeck JP. MrBayes 3.2: efficient Bayesian phylogenetic inference and model choice across a large model space. Syst Biol. 2012;61(3):539–42.View ArticlePubMedPubMed CentralGoogle Scholar

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