Next Article in Journal
Molecular and Cellular Characterization of Avian Reticulate Scales Implies the Evo–Devo Novelty of Skin Appendages in Foot Sole
Previous Article in Journal
Regionalized Protein Localization Domains in the Zebrafish Hair Cell Kinocilium
Previous Article in Special Issue
Neurogenin 2 and Neuronal Differentiation 1 Control Proper Development of the Chick Trigeminal Ganglion and Its Nerve Branches
 
 
Search for Articles:
Title / Keyword
Author / Affiliation / Email
Journal
Article Type
 
 
Advanced Search
 
Section
Special Issue
Volume
Issue
Number
Page
 
Journals
JDB
Volume 11
Issue 3
10.3390/jdb11030029
jdb-logo
Submit to this Journal Review for this Journal Propose a Special Issue
► Article Menu

Article Menu

share Share announcement Help format_quote Cite question_answer Discuss in SciProfiles thumb_up
...
Endorse textsms
...
Comment
first_page
settings
Order Article Reprints
Font Type:
Arial Georgia Verdana
Font Size:
Aa Aa Aa
Line Spacing:
Column Width:
Background:
Article

The Tumor Suppressor Adenomatous Polyposis Coli (apc) Is Required for Neural Crest-Dependent Craniofacial Development in Zebrafish

by
Xiaolei Liu
1,†,
William D. Jones
2,†,
Mathieu Quesnel-Vallières
3,
Sudhish A. Devadiga
4,
Kristin Lorent
5,
Alexander J. Valvezan
1,‡,
Rebecca L. Myers
1,
Ning Li
6,
Christopher J. Lengner
6,7,
Yoseph Barash
3,
Michael Pack
5 and
Peter S. Klein
1,2,7,*
1
Department of Medicine (Hematology-Oncology), Perelman School of Medicine, University of Pennsylvania, Philadelphia, PA 19104, USA
2
Cell and Molecular Biology Graduate Group, Perelman School of Medicine, University of Pennsylvania, Philadelphia, PA 19104, USA
3
Department of Genetics, Perelman School of Medicine, University of Pennsylvania, Philadelphia, PA 19104, USA
4
Faculty of Arts and Sciences, University of Pennsylvania, Philadelphia, PA 19104, USA
5
Department of Medicine (Gastroenterology), Perelman School of Medicine, University of Pennsylvania, Philadelphia, PA 19104, USA
6
Department of Biomedical Sciences, School of Veterinary Medicine, University of Pennsylvania, Philadelphia, PA 19104, USA
7
Department of Cell and Developmental Biology, Perelman School of Medicine, Institute for Regenerative Medicine, University of Pennsylvania, Philadelphia, PA 19104, USA
*
Author to whom correspondence should be addressed.
†
These authors contributed equally to this work.
‡
Current address: Department of Pharmacology, Robert Wood Johnson Medical School, Rutgers University, Piscataway, NJ 08854, USA.
J. Dev. Biol. 2023, 11(3), 29; https://doi.org/10.3390/jdb11030029
Submission received: 29 November 2022 / Revised: 5 June 2023 / Accepted: 9 June 2023 / Published: 29 June 2023
(This article belongs to the Special Issue From Cell to Embryo: A Theme Issue Honoring Professor Dr. Roberto Mayor)
Browse Figures
Versions Notes

Abstract

:
Neural crest (NC) is a unique vertebrate cell type arising from the border of the neural plate and epidermis that gives rise to diverse tissues along the entire body axis. Roberto Mayor and colleagues have made major contributions to our understanding of NC induction, delamination, and migration. We report that a truncating mutation of the classical tumor suppressor Adenomatous Polyposis Coli (apc) disrupts craniofacial development in zebrafish larvae, with a marked reduction in the cranial neural crest (CNC) cells that contribute to mandibular and hyoid pharyngeal arches. While the mechanism is not yet clear, the altered expression of signaling molecules that guide CNC migration could underlie this phenotype. For example, apcmcr/mcr larvae express substantially higher levels of complement c3, which Mayor and colleagues showed impairs CNC cell migration when overexpressed. However, we also observe reduction in stroma-derived factor 1 (sdf1/cxcl12), which is required for CNC migration into the head. Consistent with our previous work showing that APC directly enhances the activity of glycogen synthase kinase 3 (GSK-3) and, independently, that GSK-3 phosphorylates multiple core mRNA splicing factors, we identify 340 mRNA splicing variations in apc mutant zebrafish, including a splice variant that deletes a conserved domain in semaphorin 3f (sema3f), an axonal guidance molecule and a known regulator of CNC migration. Here, we discuss potential roles for apc in CNC development in the context of some of the seminal findings of Mayor and colleagues.

Graphical Abstract

1. Introduction

The neural crest (NC) is a remarkable vertebrate cell type induced at the border of the neural plate and adjacent epidermis. NC has the potential to develop into diverse cell types including muscle, cartilage, bone, peripheral and enteric neurons, glia, endocrine cells, melanocytes, and portions of the cardiac outflow tract, aortic arch, and semilunar valves [1,2,3,4,5,6]. The cranial neural crest (CNC) arises from the anterior neural plate border and gives rise to craniofacial muscles, cartilage, and bones as well as the cephalic peripheral nervous system, and thereby, gives rise to much of the vertebrate head and face.
Roberto Mayor and his colleagues have made major contributions to the study of NC induction, delamination, and migration and the cell biology and biomechanics of migration after NC cells leave the neural folds and move toward their diverse destinations [1,7,8,9,10,11,12,13,14,15,16,17,18]. As the neural tube closes, NC cells undergo an epithelial to mesenchymal transition (EMT), delaminate, and begin their migration throughout the body. CNC cells initiate migration as a unified group of cells, whereas trunk NC cells delaminate individually [19]. The complex sequence of instructions required for NC to undergo EMT, migration, and the eventual invasion of distant points has often been compared to the metastasis of cancer cells [4,20]. Mayor and colleagues have been pioneers in using the delamination of the NC for the in vivo study of EMT under physiological conditions.
The Mayor group has shown that, in the early phase of NC migration, cells maintain contact through several mechanisms. A seminal paper by Carmona-Fontaine et al. [10] defined an essential role for the contact inhibition of locomotion (CIL) in NC migration. CIL had been described previously as a cell behavior in which cells reorient their direction of migration upon contact with another cell [21]. Mayor, Stern, and colleagues showed that NC cells from Xenopus laevis and zebrafish depend on CIL for oriented migration; when a NC cell encounters another NC cell, it stops and reorients its direction of migration along with other NC cells. In contrast, when it encounters a different cell type, it invades that other tissue, as they showed using NC explants as well as in vivo imaging [10]. Within a migrating group of cells, the cells at the leading edge maintain greater polarity than internal cells and appear to lead directed movement, while the internal cells are primarily attracted to each other. The CNC cells of Xenopus secrete the complement factor C3, which is cleaved to generate the chemoattractive C3a polypeptide. CNC cells also express the C3a receptor [11], allowing mutual attraction, termed by the Mayor group as co-attraction (CoA). Furthermore, the overexpression of C3a diverts CNC from their normal path and impairs collective CNC cell migration, reinforcing the conclusion that C3a maintains CNC as a coherent group of cells to allow collective cell migration [11,17].
Wnt signaling plays essential and complex roles in NC development. Canonical Wnt/β-catenin signaling induces NC beginning in the gastrula stage, but this pathway must also be inhibited for the delamination of NC [13,22]. The secreted Wnt pathway inhibitor Draxin also modulates the timing of CNC EMT and migration [23]. Canonical Wnt signaling is also reduced in migrating CNC, and the ectopic activation of canonical Wnt signaling inhibits CNC cell migration [24]. Once CNC cells have arrived at their target tissues, the activation of canonical Wnt signaling promotes the differentiation of CNC, for example into chondrocytes [25].
While exploring the in vivo interplay between two Wnt pathway suppressors, Adenomatous Polyposis Coli (APC) and Glycogen Synthase Kinase 3 (GSK-3) [26,27,28], we uncovered a striking defect in the CNC contribution to craniofacial structures in apc mutant zebrafish. As presented here, this CNC defect is associated with marked elevation in c3 expression; one hypothesis to explain this defect, therefore, is that elevated c3 at an earlier stage of development in apc mutants disrupts the migration of CNC into the head, similar to the findings of Carmona-Fontaine at earlier stages of CNC migration [11]. APC is a classical tumor suppressor gene and GSK-3 is a protein kinase that phosphorylates the canonical Wnt signaling effector β-catenin. APC and GSK-3 function together to suppress the canonical Wnt signaling pathway by promoting the degradation of β-catenin. All of these proteins bind to the scaffold protein Axin, where APC directly enhances GSK-3 enzymatic activity toward β-catenin [28]. Wnt signaling is activated when an extracellular Wnt protein binds to a receptor complex and promotes the dissociation of APC from the Axin complex [28,29,30], leading to reduced GSK-3 enzymatic activity in the absence of APC.
To characterize the APC-dependent regulation of GSK-3 in more depth in vivo, we have examined the zebrafish apcmcr mutant [26], which has a truncating mutation in the mutation cluster region (mcr) that is similar to mutations associated with human colon cancers. The zebrafish apcmcr/mcr mutation is lethal in the early larva and causes multiple developmental phenotypes, including defects in heart looping, the expansion of endocardial cushions, reduced blood flow, liver hyperplasia, and the disruption of the anterior-posterior body axis [31,32]. These phenotypes are due to reduced Gsk-3 activity in the absence of full-length Apc. As a major role for GSK-3 in the Wnt pathway is to phosphorylate β-catenin and target it for degradation, some of the apc phenotypes arise through the accumulation of β-catenin [31]. However, several major phenotypes in apcmcr zebrafish are caused by the activation of other GSK-3 targets, including the nutrient sensor mechanistic target of rapamycin complex 1 (mTORC1) [26].
While examining Apc- and Gsk-3-dependent phenotypes in apcmcr mutants, we observed a highly penetrant defect that results in the accumulation of disorganized tissue just anterior to the developing heart. The examination of a CNC reporter shows marked reduction in the CNC contribution to craniofacial structures derived from the first and second pharyngeal arches along with the expansion and disorganization of CNC in more posterior pharyngeal arches. The transcriptomic comparisons of wild-type and apc mutant fish demonstrate the robust activation of canonical Wnt signaling, as expected, but also show the marked elevation of Complement Factor c3 expression, which could contribute to this aberrant CNC phenotype by interfering with or diverting the migration of CNC that normally populates the first and second pharyngeal arches. However, we also observe changes in the expression of the other regulators of both differentiation and migration that may also play a role in the CNC phenotype we report here. Because GSK-3 is a novel global regulator of mRNA splicing, we also examined splicing in apc mutant zebrafish and identified hundreds of alternative spliced mRNAs, affecting a preponderance of mRNAs that regulate cell migration, specifically in the apc mutants.

2. Methods

2.1. Zebrafish Husbandry and Methods

Embryos were raised at 28.5 °C in standard E3 medium [26,33]. apcmcr zebrafish (kindly provided by Dr. Adam Hurlstone) and primers used for genotyping were described previously [26]. The live imaging of fli1-GFP larvae was performed with an Olympus MVX10 fluorescent dissecting microscope (Tokyo, Japan). The confocal imaging of fli1-GFP larvae was performed on a Zeiss LSM 510 confocal microscope. In situ hybridization was performed on embryos and larvae fixed at the stages indicated in the figures according to well-described methods [34]. Probes included gsc, crestin, sox10. Plasmids for gsc and crestin were kindly provided by Dr. Mary Mullins (University of Pennsylvania School of Medicine). For sox10 in situ hybridization, an 832 bp fragment of sox10 was PCR amplified with the primers GTCACTAAAGGTCCAACCGT and TGTGATGGACTTGAGGCACT and the product was subcloned into pCRII-TOPO; this plasmid was used as a template for the in vitro transcription of in situ hybridization probes. Zebrafish husbandry and egg procurement were carried out in accordance with the guidelines of the University of Pennsylvania Institutional Animal Care and Use Committee.

2.2. RNA Isolation, RT-PCR, and Sequencing

apcmcr/mcr homozygous embryos were sorted from wild-type and apcmcr/+ heterozygotes based on morphology (homozygotes displayed a bent A–P axes, whereas heterozygotes were morphologically indistinguishable from WT) at 24 h post-fertilization (hpf) and harvested for RNA isolation at 48 hpf. A total of 20 embryos per genotype were collected from 3 independent clutches, and RNA was isolated using Trizol reagent, as described previously [35]. Genomic DNA was removed via DNAse treatment and total RNA was recovered using an RNeasy kit (Qiagen, Germantown, MD, USA). Purity was confirmed via a bioanalyzer (RIN > 8). RNAs were sent to Genewiz for polyA-selection, for the generation of stranded Illumina RNA-Seq library, and for sequencing at a depth of ≥50 million reads per sample replicate. For standard qRT-PCR, 50 ng RNA per sample was used for first-strand cDNA synthesis using SuperScript-III reverse transcriptase (Invitrogen, Waltham, MA, USA), according to manufacturer’s protocol. Relative gene expression was quantified by real-time PCR using Power Sybr Green PCR Master Mix, as described [36]. GAPDH was used as a control for RNA input. PCR primer sequences are shown in Table 1.

2.3. Quantification of Alternative Spliced and Differentially Expressed Genes

Alternative splicing and differential expression analyses were based on RNA-Seq reads that were mapped to the zebrafish reference genome (GRCz10) using STAR (https://www.ncbi.nlm.nih.gov/pmc/articles/PMC3530905/, accessed on 15 January 2018). Differential splicing analysis was performed comparing WT/het and apcmcr/mcr samples using Modeling Alternative Junction Inclusion Quantification (MAJIQ) deltapsi with intron retention quantification enabled. Results were filtered for high confidence changing local splice variants (LSVs) with a change in percent spliced in (dPSI) ≥20% (in which junctions had a ≥90% probability of expected dPSI).

2.4. Statistical Analysis and Downstream Bioinformatics

The results are presented as mean ± SD. Unpaired two-tailed Student’s t-tests were applied RT-qPCR data to determine differences in mRNA expression. p values were calculated following log2 transformation. Gene expression data from RNA-seq were obtained by aligning poly-A reads to the zebrafish reference genome (GRCz10) using STAR as described previously [35]. The generation of heatmaps and clustering analyses were performed using Morpheus (https://software.broadinstitute.org/morpheus/, accessed 22 March 2019). GO and KEGG (Kyoto Encyclopedia of Genes and Genomes) pathway analysis were performed using Metascape [37]. The list of genes that changed ≥2-fold with FDR <0.05 in apcmcr/mcr mutants vs. combined WT and apcmcr/+ heterozygotes was submitted as the gene list. For Gene Set Enrichment Analysis (GSEA), Zebrafish Information Network (ZFIN) gene IDs were converted to homologous human gene symbols in Ensembl version 95 using the Bioconductor biomaRt package for Ensembl BioMart [38,39,40] and this list was submitted to GSEA 4.3.2 (https://www.gsea-msigdb.org/gsea/index.jsp, accessed 26 November 2022) to determine enriched pathways [41,42] Supplemental Table S3 shows GSEA identified Hallmark pathways ranked by normalized enrichment score.

3. Results

3.1. The Tumor Suppressor Apc Is Required for the CNC Contribution to Craniofacial Structures

Defects in morphogenesis leading to curvature of the anterior–posterior axis are a prominent feature of the apcmcr mutant [26,31]. This phenotype is detectable as early as 24 hpf, and by 50 hpf (~30 somites), it is associated with a collection of amorphous tissue anterior to the yolk mass and developing heart (Figure 1A–D). As the identity of the cells contributing to this aberrant tissue mass was not clear, we crossed apcmcr mutants with reporter lines that express GFP in vascular endothelial cells (fli1-GFP) [43], renal tubular epithelium (enpep-GFP), gut endoderm (foxa3-GFP), and smooth muscle (sm22alpha-GFP). Although most tissue-specific markers showed relatively normal expression patterns within the region of interest, fli1-GFP; apcmcr mutant larvae showed a high accumulation of GFP+ cells within these amorphic cell clusters and markedly reduced GFP+ cells in the ventral head (Figure 1E). fli1-GFP is expressed in vascular endothelium throughout the larva and in CNC-derived pharyngeal arch mesenchyme [43]. Confocal imaging showed that Fli1-GFP+ expression is similar in the vascular structures of the trunk in wild-type (WT) and apcmcr mutants (Figure 1F,G). In stark contrast, GFP+ cells that are prominent in craniofacial structures derived from the first and second pharyngeal arches in wild-type larvae, including Meckel’s cartilage, the palatoquadrate cartilage, and the ceratohyal cartilage (Figure 1H), are markedly reduced or absent in apc mutants. These reductions are accompanied by an increased number and disorganization of Fli1-GFP+ cells within more posterior pharyngeal arches (Figure 1I), corresponding to the aberrant cell cluster we observe in intact larvae and by histological sectioning (Figure 1B,D). The low level of GFP+ cells present in the heads of apcmcr mutants may reflect reduced vascular endothelial and/or CNC cells.
The absence of CNC cells in the derivatives of the mandibular and hyoid arches could reflect the disruption of CNC specification or migration. However, this defect is not caused by a disruption of initial NC induction, as the expression of the early NC marker sox10 at the neural plate border is normal in apc mutants at the 5-somite stage (12 hpf; Figure 2A,B). The overall level of expression of the pan-NC marker crestin was also similar in WT and apcmcr larvae at 33 hpf. However, at later stages of larval development (55 hpf), the paired-like homeobox transcription factor goosecoid (gsc), which is highly expressed in the mandibular, hyoid, and more posterior pharyngeal arches in WT larvae (Figure 2C, [44]), was absent from these CNC-derived structures in apcmcr mutant larvae (Figure 2D). The reduced expression of gsc in apcmcr mutants was also observed via RNA-seq, as described below (Figure 3). These findings demonstrate a marked defect in craniofacial development in apcmcr mutants that we hypothesize was caused by a failure of CNC to migrate into the head, although, alternatively, altered cell fate specification could still underlie this defect as well.

3.2. Increased Expression of Cytokines and Wnt Target Genes in apcmcr/mcr Larvae

To gain a deeper understanding of how Apc regulates the expression of genes that may influence CNC specification and/or migration, as well as more general insights into the role of APC in global gene expression, we performed RNA sequencing (RNA-seq) on the wild-type and apc mutant larvae at 48 hpf. RNA-seq was performed with three biological replicates and sequenced at a depth of ≥50 million reads per sample. Using a threshold of ≥ 2-fold change and false discovery rate (FDR) < 0.05, we observed the increased abundance of 918 mRNAs and the decreased abundance of 881 mRNAs in the apcmcr mutant compared to wild-type larvae (Figure 3A and Supplemental Table S1).
The expression of >30 established Wnt target genes and Wnt-inducible pathway antagonists, including c-myc, dickkopf 1 (dkk1), dkk2, naked cuticle homologs 1–3 (nkd1–3), notum 1, R-spondin 2 (rspo2), axin2, myc, apc downregulated 1 (apcdd1), wnt1 inducible signaling pathway protein 1 (wisp1), wnt inhibitory factor 1 (wif1), sp5, engrailed2 (en2), and twist1, was robustly increased in apcmcr mutant larvae, as expected. The visual inspection of this list also revealed an increase in mRNA abundance for many inflammatory cytokines, cytokine receptors, and mediators of cytokine signaling, including ccl19a, interleukin 11 (il11), leptin, parathyroid hormone 1, suppressor of cytokine signaling 3 (socs3), cxcl19, angiopoietin 2, colony stimulatory factor 1 (csf1), and others (Supplemental Table S1). To validate changes in RNA abundance observed by RNA-seq, we performed RT-qPCR on selected genes and found close correlation using the two methods for all genes tested (Figure 3B). These data confirm the increased expression of cytokines, Wnt target genes, and Wnt antagonists. In contrast, the expression of gsc was reduced by greater than five-fold, consistent with the marked reduction in gsc expression observed by in situ hybridization (Figure 2D).
To identify the patterns of gene expression changes in apcmcr mutants, we performed gene ontology (GO) analysis using Metascape [37]. In addition to confirming the altered expression of Wnt target genes and inflammatory cytokines, this analysis revealed significant changes in the expression of genes related to cell migration, extracellular matrix organization, cell fate specification, and cartilage development (Figure 3C), consistent with alterations in CNC migration, differentiation, and craniofacial development. The reduced expression at 48 hpf of genes enriched in cartilage, including foxl1, loxl2b, and2, tfap2b, and col11a2 (Supplemental Table S1), is consistent with the loss of CNC-derived craniofacial cartilages in apcmcr mutant larvae.

3.3. Increased Expression of Complement c3 in apcmcr/mcr Larvae

Mayor and colleagues showed that the complement C3 cleavage product C3a mediates the mutual attraction of CNC cells when they are migrating as a group and that the overexpression of C3a misdirects and impairs collective CNC cell migration. Consistent with the hypothesis that the CNC defect we observe could be due to disrupted CNC migration, we find the significantly elevated expression of c3 genes in apcmcr larvae at 48 hpf (Figure 3D,E). While Carmona-Fontaine et al. examined CNC migration at an earlier stage following delamination [11], it is likely that C3a is also required for collective CNC cell migration at later stages and thus elevated c3 expression at later stages may also interfere with CNC migration into the head. Gene set enrichment analysis (GSEA [41]) identified the upregulation of additional genes associated with the complement pathway and EMT (Figure 3F), as well as c-Myc, Wnt/β-catenin, and mTORC1 signaling pathways, as expected with an apc loss of function mutation (Supplemental Table S3).
These findings are consistent with the hypothesis that the migration of CNC cells into the head is disrupted in apc mutants by the overexpression of c3 genes. However, we also observe changes in the expression of other secreted factors that have been shown to function as CNC chemoattractants or repellents. For example, the expression of stromal-derived Factor 1 (sdf1)/cxcl12, which is expressed in pharyngeal endoderm [46] and is required for CNC migration into the head in zebrafish, Xenopus, and other organisms [16,46,47], is reduced 2.5-fold in apcmcr mutant larvae. In addition, multiple semaphorin family genes, axonal guidance molecules that can also instruct the direction of NC migration, show significantly altered expression in apcmcr larvae (Figure 3D). It should also be pointed out that the RNA-seq analysis was performed at 48 hpf, within the window of CNC differentiation, whereas CNC migration primarily occurs at earlier stages.

3.4. An Oncogenic apc Mutation Alters mRNA Splicing

APC enhances the activity of GSK-3, and therefore, GSK-3 activity is reduced by oncogenic apc mutations, including the apcmcr mutation in zebrafish [26,28]. The inhibition of GSK-3 reduces the phosphorylation of multiple splicing factors in diverse mammalian cell types and alters the splicing of hundreds of mRNAs in mammalian cells [35,48,49,50]. Germline mutations in splicing factors are associated with craniofacial defects in humans and mice [51,52]. As somatic mutations in splicing factors are also associated with multiple solid and hematologic malignancies [53,54], we hypothesized that the reduced GSK-3 activity associated with oncogenic apc mutations might also disrupt mRNA splicing. We therefore analyzed the above RNA-seq dataset for splicing changes in apcmcr mutant zebrafish using the MAJIQ pipeline [55]. For a fractional change in splicing (change in percent spliced in or ∆PSI) ≥0.20 with a probability >0.90, we identified 340 splicing variations in apcmcr larvae compared to wild-type larvae (Figure 4A, Supplemental Table S2). Alternative splicing events included exon skipping, alternative 5′ and alternative 3′ splice sites, and other splicing changes (Figure 4B). GO analysis identified splicing variations in mRNAs encoding regulators of cell adhesion, cell migration, cytoskeleton, and cell morphogenesis (Figure 4C).
We also observed the significantly altered splicing of the “a” allele of semaphorin 3f (sema3fa; Figure 4D,E), a secreted axonal guidance molecule that is required for CNC migration in mice and chickens [56,57]. Under control conditions, sema3fa mRNA predominantly includes exon 6 with less than 8% of transcripts alternatively spliced to skip this exon. In apcmcr mutants, 35.4% of transcripts skip exon 6, deleting a sequence within the highly conserved sema domain and generating a transcript predicted to encode a nonfunctional protein. Although we have not tested whether these changes have functional consequences, the data nevertheless make it clear that oncogenic mutations in apc can markedly alter the splicing of multiple mRNAs across the transcriptome, including mRNAs known to regulate CNC migration.

4. Discussion

NC comprises a unique and complex set of multipotent cells that undergo induction, migration, invasion, and differentiation into diverse cell types. Roberto Mayor and his colleagues have made seminal contributions to our understanding of NC induction and migration [1,7,8,9,10,11,12,13,14,15,16,17,18]. Their elucidation of collective cell movements during CNC migration and the role of C3 in mediating the co-attraction of migrating CNC cells suggests the hypothesis that the marked reduction in CNC cells in the head of apcmcr/mcr larvae could be due to elevated c3 expression disrupting or misdirecting the migration of CNC cells that normally populate the first and second pharyngeal arches. However, we also observe robust changes in the expression of other factors that guide CNC migration and that could contribute to the CNC defect in apcmcr zebrafish. Importantly, our data do not rule out the possibility that the defect is primarily due to a change in CNC cell fate specification, despite the normal expression of pan-NC markers sox10 and crestin. Similarly, the reduced expression of sdf1 raises the possibility that the defects in the mandibular and hyoid arches is caused by altered development of pharyngeal endoderm [46]. While future research will need to examine CNC cells during the migration phase of NC development, the morphological data reported here nevertheless define a novel and dramatic CNC phenotype caused by an apc loss of function mutation. Furthermore, our transcriptomic data suggest testable hypotheses for the role of secreted molecules, such as C3, Sdf1, and Sema3f, as downstream targets of APC in the regulation of CNC migration.
The striking absence of gsc expression in the mandibular and hyoid arches of apcmcr larvae is reminiscent of the human neurocristopathy SAMS (short stature, auditory-canal atresia, mandibular hypoplasia, and skeletal abnormalities) that has been associated with GSC mutations [58] and is consistent with knockout data in mice showing that gsc is required for craniofacial development [59,60].
In humans, APC is a classical tumor suppressor gene that is mutated in most cases of colorectal carcinomas. Although neoplasia associated with APC mutation is generally ascribed to the activation of canonical Wnt/β-catenin target genes, APC suppresses other downstream targets, and these are also activated by an APC loss of function mutations. As APC directly enhances GSK-3 activity, the loss of APC reduces GSK-3 activity and activates downstream effectors that are normally inhibited by GSK-3, such as mTORC1. Indeed, multiple apcmcr phenotypes are reversed by inhibiting mTORC1 [26]. Thus, the CNC/craniofacial defect we observe with apc loss may also arise through a GSK-3-dependent but β-catenin-independent mechanism. In support of this hypothesis, conditional KO of Gsk3 in mice causes pronounced craniofacial defects independently of β-catenin [61].
GSK-3 phosphorylates multiple splicing factors and regulates mRNA splicing at a genome-wide level [35,48,49,50]. Thus, we predicted that loss of apc would also disrupt splicing by impairing GSK-3 activity. Indeed, the apcmcr/mcr mutation significantly alters the usage of 340 splicing variations. Alternatively spliced mRNAs included sema3f, which has previously been shown to mediate CNC migration [56] and other genes involved in cell migration. The broad disruption of alternative splicing in apcmcr mutants suggests a parallel with a group of disorders referred to as craniofacial spliceosomopathies [51,52,62]. Alternative splicing is tightly regulated spatially and temporally during craniofacial development in the mouse in a manner that correlates with the changes in the expression of RNA-binding proteins [62]. Furthermore, multiple human disorders in craniofacial development are associated with germline mutations in splicing factors, spliceosome assembly factors, and other RNA-binding proteins, including PUF60, EFTUD2, SF3B4, SNRPB, SNRPA, EIF4A3, TXNL4A, RBM8A, HNRNPR, RBM10, and HRNNPH2 [51,52,62,63,64]. Thus, the defect in craniofacial development in apcmcr mutant zebrafish could similarly arise through the disruption of alternative splicing regulated by GSK-3. Future studies will address whether apc-dependent splicing variations are mediated through GSK-3 and whether the alternative splicing of sema3f alters CNC migration or otherwise contributes to the craniofacial phenotype in apcmcr mutants. We also suggest the hypothesis that alternative splicing caused by the APC loss of function could contribute to the malignant phenotypes associated with APC-related cancers.
NC migration has been frequently compared to the metastasis of epithelial cancers [6,17,18,20]. In both cases, the cells exit their initial locations through EMT mediated by the increased expression of Snail family transcription factors and the down-regulation of epithelial cell adhesion molecules, such as E-Cadherin. Upon delamination, CNC cells undergo collective cell migration, as described by Mayor’s group, in a manner that is similar to more recent observations in pancreatic, colorectal, and breast cancers, in which tumor cells undergo “partial EMT” (p-EMT) and then migrate collectively as cell clusters before invading their final destinations [65,66,67,68]. Similar to CNC, ovarian cancer cells secrete C3, which is induced in these cells by the EMT factor Twist1 and is expressed at the invasive edge of metastatic cells in vivo [69]. We observe the increased expression of twist1 in the apcmcr mutant larvae, and this could also contribute to the increase in c3a expression. Thus, C3 could serve a similar function in APC-related cancers by maintaining the association of metastatic cells in transit.

5. Conclusions

In summary, we report that a truncating mutation in the tumor suppressor gene apc in zebrafish disrupts CNC-dependent craniofacial development. The deep sequencing of expressed RNAs reveals the increased expression of complement c3 in apc mutant larvae. Based on the seminal work of Mayor and colleagues, showing that C3 overexpression impairs CNC migration, we propose the testable hypothesis that the overexpression of c3 caused by the loss of apc disrupts or misdirects CNC migration into the head. However, the apcmcr mutation also alters the expression of other important mediators of CNC migration, including the reduced expression of SDF1/CXCL12 and varied effects on multiple semaphorin family members. These changes in expression or altered cell fate not identified by sox10 or crestin expression analysis could alternatively be responsible for the marked craniofacial defects we observe in apcmcr larvae. Finally, we show that Apc significantly regulates the splicing of hundreds of mRNAs, including sema3f. We propose that this is through the direct modulation of GSK-3 activity and that disrupted splicing associated with APC loss of function mutations may contribute to craniofacial defects during zebrafish development as well as the pathogenesis of colon cancer in humans. These data provide a basis for future studies into the roles of APC, GSK-3, and mRNA splicing in cell migration and fate specification in normal development and in cancer metastasis.

Supplementary Materials

The following supporting information can be downloaded at: https://www.mdpi.com/article/10.3390/jdb11030029/s1, Supplemental Table S1: RNA-seq apc vs. wt; Supplemental Table S2: splicing analysis; Supplemental Table S3: GSEA.

Author Contributions

Conceptualization, X.L., P.S.K., W.D.J., M.Q.-V. and Y.B.; methodology, X.L., W.D.J., M.Q.-V. and K.L.; validation, X.L. and W.D.J.; investigation, X.L., W.D.J., M.Q.-V., S.A.D., K.L., A.J.V., R.L.M., N.L., C.J.L., Y.B., M.P. and P.S.K.; resources, Y.B., M.P., and P.S.K.; data curation, X.L., W.D.J. and M.Q.-V.; writing—original draft preparation, P.S.K. and X.L.; writing—review and editing, X.L., W.D.J., M.Q.-V., N.L., C.J.L., R.L.M., Y.B. and P.S.K.; visualization, X.L., W.D.J., K.L. and A.J.V.; supervision, P.S.K.; funding acquisition, P.S.K. and Y.B. All authors have read and agreed to the published version of the manuscript.

Funding

This research was supported by National Institutes of Health grants to P.S.K. (R01GM115517; R56DK133258-01) and to Y.B. (U01CA232563) and a grant from the Leukemia and Lymphoma Society to P.S.K. (LLS#8036-23).

Institutional Review Board Statement

Zebrafish experiments were carried out in accordance with the guidelines of the University of Pennsylvania Institutional Animal Care and Use Committee (IACUC protocol # 804887). This study did not involve humans or human tissues.

Informed Consent Statement

Not applicable.

Data Availability Statement

RNA-seq data were deposited in the NCBI Gene Expression Omnibus [70] and are accessible through GEO Series accession number GSE234986. (https://www.ncbi.nlm.nih.gov/geo/query/acc.cgi?acc=GSE234986).

Acknowledgments

We thank Kristin Artinger, Jean-Pierre Saint-Jeannet, Arndt Siekmann, Kristen Lynch, and Robert Heuckeroth for helpful discussions and Mary Mullins for plasmids. We also thank Andrea Stout and the Cell and Developmental Biology Imaging Core for help with confocal imaging and John Tobias for bioinformatics support.

Conflicts of Interest

The authors declare no conflict of interest.

References

  1. Aybar, M.J.; Mayor, R. Early induction of neural crest cells: Lessons learned from frog, fish and chick. Curr. Opin. Genet. Dev. 2002, 12, 452–458. [Google Scholar] [CrossRef]
  2. Jain, R.; Rentschler, S.; Epstein, J.A. Notch and cardiac outflow tract development. Ann. N. Y. Acad. Sci. 2010, 1188, 184–190. [Google Scholar] [CrossRef] [Green Version]
  3. LaBonne, C.; Bronner-Fraser, M. Snail-related transcriptional repressors are required in Xenopus for both the induction of the neural crest and its subsequent migration. Dev. Biol. 2000, 221, 195–205. [Google Scholar] [CrossRef] [Green Version]
  4. Mayor, R.; Theveneau, E. The neural crest. Development 2013, 140, 2247–2251. [Google Scholar] [CrossRef] [Green Version]
  5. Shellard, A.; Mayor, R. Chemotaxis during neural crest migration. Semin. Cell Dev. Biol. 2016, 55, 111–118. [Google Scholar] [CrossRef] [PubMed]
  6. Klymkowsky, M.W.; Rossi, C.C.; Artinger, K.B. Mechanisms driving neural crest induction and migration in the zebrafish and Xenopus laevis. Cell Adh. Migr. 2010, 4, 595–608. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  7. Bajanca, F.; Gouignard, N.; Colle, C.; Parsons, M.; Mayor, R.; Theveneau, E. In vivo topology converts competition for cell-matrix adhesion into directional migration. Nat. Commun. 2019, 10, 1518. [Google Scholar] [CrossRef] [Green Version]
  8. Barriga, E.H.; Franze, K.; Charras, G.; Mayor, R. Tissue stiffening coordinates morphogenesis by triggering collective cell migration in vivo. Nature 2018, 554, 523–527. [Google Scholar] [CrossRef]
  9. Canales Coutino, B.; Mayor, R. The mechanosensitive channel Piezo1 cooperates with semaphorins to control neural crest migration. Development 2021, 148, dev200001. [Google Scholar] [CrossRef] [PubMed]
  10. Carmona-Fontaine, C.; Matthews, H.K.; Kuriyama, S.; Moreno, M.; Dunn, G.A.; Parsons, M.; Stern, C.D.; Mayor, R. Contact inhibition of locomotion in vivo controls neural crest directional migration. Nature 2008, 456, 957–961. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  11. Carmona-Fontaine, C.; Theveneau, E.; Tzekou, A.; Tada, M.; Woods, M.; Page, K.M.; Parsons, M.; Lambris, J.D.; Mayor, R. Complement fragment C3a controls mutual cell attraction during collective cell migration. Dev. Cell 2011, 21, 1026–1037. [Google Scholar] [CrossRef] [Green Version]
  12. Mancilla, A.; Mayor, R. Neural crest formation in Xenopus laevis: Mechanisms of Xslug induction. Dev. Biol. 1996, 177, 580–589. [Google Scholar] [CrossRef] [Green Version]
  13. Rabadan, M.A.; Herrera, A.; Fanlo, L.; Usieto, S.; Carmona-Fontaine, C.; Barriga, E.H.; Mayor, R.; Pons, S.; Marti, E. Delamination of neural crest cells requires transient and reversible Wnt inhibition mediated by Dact1/2. Development 2016, 143, 2194–2205. [Google Scholar] [CrossRef] [Green Version]
  14. Shellard, A.; Mayor, R. Collective durotaxis along a self-generated stiffness gradient in vivo. Nature 2021, 600, 690–694. [Google Scholar] [CrossRef]
  15. Shellard, A.; Szabo, A.; Trepat, X.; Mayor, R. Supracellular contraction at the rear of neural crest cell groups drives collective chemotaxis. Science 2018, 362, 339–343. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  16. Theveneau, E.; Marchant, L.; Kuriyama, S.; Gull, M.; Moepps, B.; Parsons, M.; Mayor, R. Collective chemotaxis requires contact-dependent cell polarity. Dev. Cell 2010, 19, 39–53. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  17. Szabo, A.; Mayor, R. Mechanisms of Neural Crest Migration. Annu. Rev. Genet. 2018, 52, 43–63. [Google Scholar] [CrossRef]
  18. Theveneau, E.; Mayor, R. Neural crest delamination and migration: From epithelium-to-mesenchyme transition to collective cell migration. Dev. Biol. 2012, 366, 34–54. [Google Scholar] [CrossRef] [Green Version]
  19. Theveneau, E.; Duband, J.L.; Altabef, M. Ets-1 confers cranial features on neural crest delamination. PLoS ONE 2007, 2, e1142. [Google Scholar] [CrossRef]
  20. Nieto, M.A. Epithelial plasticity: A common theme in embryonic and cancer cells. Science 2013, 342, 1234850. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  21. Abercrombie, M.; Heaysman, J.E. Observations on the social behaviour of cells in tissue culture. I. Speed of movement of chick heart fibroblasts in relation to their mutual contacts. Exp. Cell Res. 1953, 5, 111–131. [Google Scholar] [CrossRef]
  22. Ji, Y.; Hao, H.; Reynolds, K.; McMahon, M.; Zhou, C.J. Wnt Signaling in Neural Crest Ontogenesis and Oncogenesis. Cells 2019, 8, 1173. [Google Scholar] [CrossRef] [Green Version]
  23. Hutchins, E.J.; Bronner, M.E. Draxin acts as a molecular rheostat of canonical Wnt signaling to control cranial neural crest EMT. J. Cell Biol. 2018, 217, 3683–3697. [Google Scholar] [CrossRef] [Green Version]
  24. Maj, E.; Kunneke, L.; Loresch, E.; Grund, A.; Melchert, J.; Pieler, T.; Aspelmeier, T.; Borchers, A. Controlled levels of canonical Wnt signaling are required for neural crest migration. Dev. Biol. 2016, 417, 77–90. [Google Scholar] [CrossRef]
  25. Shull, L.C.; Lencer, E.S.; Kim, H.M.; Goyama, S.; Kurokawa, M.; Costello, J.C.; Jones, K.; Artinger, K.B. PRDM paralogs antagonistically balance Wnt/beta-catenin activity during craniofacial chondrocyte differentiation. Development 2022, 149, dev200082. [Google Scholar] [CrossRef] [PubMed]
  26. Valvezan, A.J.; Huang, J.; Lengner, C.J.; Pack, M.; Klein, P.S. Oncogenic mutations in adenomatous polyposis coli (Apc) activate mechanistic target of rapamycin complex 1 (mTORC1) in mice and zebrafish. Dis. Model. Mech. 2014, 7, 63–71. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  27. Valvezan, A.J.; Klein, P.S. GSK-3 and Wnt Signaling in Neurogenesis and Bipolar Disorder. Front. Mol. Neurosci. 2012, 5, 1. [Google Scholar] [CrossRef] [Green Version]
  28. Valvezan, A.J.; Zhang, F.; Diehl, J.A.; Klein, P.S. Adenomatous polyposis coli (APC) regulates multiple signaling pathways by enhancing glycogen synthase kinase-3 (GSK-3) activity. J. Biol. Chem. 2012, 287, 3823–3832. [Google Scholar] [CrossRef] [Green Version]
  29. Ji, L.; Lu, B.; Wang, Z.; Yang, Z.; Reece-Hoyes, J.; Russ, C.; Xu, W.; Cong, F. Identification of ICAT as an APC Inhibitor, Revealing Wnt-Dependent Inhibition of APC-Axin Interaction. Mol. Cell 2018, 72, 37–47.e34. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  30. Tran, H.; Polakis, P. Reversible modification of adenomatous polyposis coli (APC) with K63-linked polyubiquitin regulates the assembly and activity of the beta-catenin destruction complex. J. Biol. Chem. 2012, 287, 28552–28563. [Google Scholar] [CrossRef] [Green Version]
  31. Hurlstone, A.F.; Haramis, A.P.; Wienholds, E.; Begthel, H.; Korving, J.; Van Eeden, F.; Cuppen, E.; Zivkovic, D.; Plasterk, R.H.; Clevers, H. The Wnt/beta-catenin pathway regulates cardiac valve formation. Nature 2003, 425, 633–637. [Google Scholar] [CrossRef] [PubMed]
  32. Goessling, W.; North, T.E.; Lord, A.M.; Ceol, C.; Lee, S.; Weidinger, G.; Bourque, C.; Strijbosch, R.; Haramis, A.P.; Puder, M.; et al. APC mutant zebrafish uncover a changing temporal requirement for wnt signaling in liver development. Dev. Biol. 2008, 320, 161–174. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  33. Westerfield, M. The Zebrafish Book a Guide for the Laboratory Use of Zebrafish Danio (Brachydanio) Rerio; Institute of Neuroscience, University of Oregon: Eugene, OR, USA, 1993. [Google Scholar]
  34. Thisse, C.; Thisse, B. High-resolution in situ hybridization to whole-mount zebrafish embryos. Nat. Protoc. 2008, 3, 59–69. [Google Scholar] [CrossRef] [PubMed]
  35. Shinde, M.Y.; Sidoli, S.; Kulej, K.; Mallory, M.J.; Radens, C.M.; Reicherter, A.L.; Myers, R.L.; Barash, Y.; Lynch, K.W.; Garcia, B.A.; et al. Phosphoproteomics reveals that glycogen synthase kinase-3 phosphorylates multiple splicing factors and is associated with alternative splicing. J. Biol. Chem. 2017, 292, 18240–18255. [Google Scholar] [CrossRef] [Green Version]
  36. Nguyen-McCarty, M.; Klein, P.S. Autophagy is a signature of a signaling network that maintains hematopoietic stem cells. PLoS ONE 2017, 12, e0177054. [Google Scholar] [CrossRef] [Green Version]
  37. Zhou, Y.; Zhou, B.; Pache, L.; Chang, M.; Khodabakhshi, A.H.; Tanaseichuk, O.; Benner, C.; Chanda, S.K. Metascape provides a biologist-oriented resource for the analysis of systems-level datasets. Nat. Commun. 2019, 10, 1523. [Google Scholar] [CrossRef] [Green Version]
  38. Durinck, S.; Spellman, P.T.; Birney, E.; Huber, W. Mapping identifiers for the integration of genomic datasets with the R/Bioconductor package biomaRt. Nat. Protoc. 2009, 4, 1184–1191. [Google Scholar] [CrossRef] [Green Version]
  39. Cunningham, F.; Allen, J.E.; Allen, J.; Alvarez-Jarreta, J.; Amode, M.R.; Armean, I.M.; Austine-Orimoloye, O.; Azov, A.G.; Barnes, I.; Bennett, R.; et al. Ensembl 2022. Nucleic Acids Res. 2022, 50, D988–D995. [Google Scholar] [CrossRef]
  40. Durinck, S.; Moreau, Y.; Kasprzyk, A.; Davis, S.; De Moor, B.; Brazma, A.; Huber, W. BioMart and Bioconductor: A powerful link between biological databases and microarray data analysis. Bioinformatics 2005, 21, 3439–3440. [Google Scholar] [CrossRef] [Green Version]
  41. Subramanian, A.; Tamayo, P.; Mootha, V.K.; Mukherjee, S.; Ebert, B.L.; Gillette, M.A.; Paulovich, A.; Pomeroy, S.L.; Golub, T.R.; Lander, E.S.; et al. Gene set enrichment analysis: A knowledge-based approach for interpreting genome-wide expression profiles. Proc. Natl. Acad. Sci. USA 2005, 102, 15545–15550. [Google Scholar] [CrossRef] [Green Version]
  42. Mootha, V.K.; Lindgren, C.M.; Eriksson, K.F.; Subramanian, A.; Sihag, S.; Lehar, J.; Puigserver, P.; Carlsson, E.; Ridderstrale, M.; Laurila, E.; et al. PGC-1alpha-responsive genes involved in oxidative phosphorylation are coordinately downregulated in human diabetes. Nat. Genet. 2003, 34, 267–273. [Google Scholar] [CrossRef] [PubMed]
  43. Lawson, N.D.; Weinstein, B.M. In vivo imaging of embryonic vascular development using transgenic zebrafish. Dev. Biol. 2002, 248, 307–318. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  44. Schulte-Merker, S.; Hammerschmidt, M.; Beuchle, D.; Cho, K.W.; De Robertis, E.M.; Nusslein-Volhard, C. Expression of zebrafish goosecoid and no tail gene products in wild-type and mutant no tail embryos. Development 1994, 120, 843–852. [Google Scholar] [CrossRef] [PubMed]
  45. Nusse, R. The Wnt Gene Homepage. 1999. Available online: http://www.stanford.edu/~rnusse/wntwindow.html (accessed on 15 February 2019).
  46. Olesnicky Killian, E.C.; Birkholz, D.A.; Artinger, K.B. A role for chemokine signaling in neural crest cell migration and craniofacial development. Dev. Biol. 2009, 333, 161–172. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  47. Belmadani, A.; Tran, P.B.; Ren, D.; Assimacopoulos, S.; Grove, E.A.; Miller, R.J. The chemokine stromal cell-derived factor-1 regulates the migration of sensory neuron progenitors. J. Neurosci. 2005, 25, 3995–4003. [Google Scholar] [CrossRef] [Green Version]
  48. Heyd, F.; Lynch, K.W. Phosphorylation-dependent regulation of PSF by GSK3 controls CD45 alternative splicing. Mol. Cell 2010, 40, 126–137. [Google Scholar] [CrossRef] [Green Version]
  49. Hernandez, F.; Perez, M.; Lucas, J.J.; Mata, A.M.; Bhat, R.; Avila, J. Glycogen synthase kinase-3 plays a crucial role in tau exon 10 splicing and intranuclear distribution of SC35. Implications for Alzheimer’s disease. J. Biol. Chem. 2004, 279, 3801–3806. [Google Scholar] [CrossRef] [Green Version]
  50. Wang, S.B.; Venkatraman, V.; Crowgey, E.L.; Liu, T.; Fu, Z.; Holewinski, R.; Ranek, M.; Kass, D.A.; O’Rourke, B.; Van Eyk, J.E. Protein S-Nitrosylation Controls Glycogen Synthase Kinase 3beta Function Independent of Its Phosphorylation State. Circ. Res. 2018, 122, 1517–1531. [Google Scholar] [CrossRef]
  51. Beauchamp, M.C.; Alam, S.S.; Kumar, S.; Jerome-Majewska, L.A. Spliceosomopathies and neurocristopathies: Two sides of the same coin? Dev. Dyn. 2020, 249, 924–945. [Google Scholar] [CrossRef]
  52. Griffin, C.; Saint-Jeannet, J.P. Spliceosomopathies: Diseases and mechanisms. Dev. Dyn. 2020, 249, 1038–1046. [Google Scholar] [CrossRef] [PubMed]
  53. Kandoth, C.; McLellan, M.D.; Vandin, F.; Ye, K.; Niu, B.; Lu, C.; Xie, M.; Zhang, Q.; McMichael, J.F.; Wyczalkowski, M.A.; et al. Mutational landscape and significance across 12 major cancer types. Nature 2013, 502, 333–339. [Google Scholar] [CrossRef] [Green Version]
  54. Cherry, S.; Lynch, K.W. Alternative splicing and cancer: Insights, opportunities, and challenges from an expanding view of the transcriptome. Genes Dev. 2020, 34, 1005–1016. [Google Scholar] [CrossRef]
  55. Vaquero-Garcia, J.; Barrera, A.; Gazzara, M.R.; Gonzalez-Vallinas, J.; Lahens, N.F.; Hogenesch, J.B.; Lynch, K.W.; Barash, Y. A new view of transcriptome complexity and regulation through the lens of local splicing variations. Elife 2016, 5, e11752. [Google Scholar] [CrossRef] [PubMed]
  56. Gammill, L.S.; Gonzalez, C.; Bronner-Fraser, M. Neuropilin 2/semaphorin 3F signaling is essential for cranial neural crest migration and trigeminal ganglion condensation. Dev. Neurobiol. 2007, 67, 47–56. [Google Scholar] [CrossRef]
  57. Osborne, N.J.; Begbie, J.; Chilton, J.K.; Schmidt, H.; Eickholt, B.J. Semaphorin/neuropilin signaling influences the positioning of migratory neural crest cells within the hindbrain region of the chick. Dev. Dyn. 2005, 232, 939–949. [Google Scholar] [CrossRef]
  58. Parry, D.A.; Logan, C.V.; Stegmann, A.P.; Abdelhamed, Z.A.; Calder, A.; Khan, S.; Bonthron, D.T.; Clowes, V.; Sheridan, E.; Ghali, N.; et al. SAMS, a syndrome of short stature, auditory-canal atresia, mandibular hypoplasia, and skeletal abnormalities is a unique neurocristopathy caused by mutations in Goosecoid. Am. J. Hum. Genet. 2013, 93, 1135–1142. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  59. Rivera-Perez, J.A.; Mallo, M.; Gendron-Maguire, M.; Gridley, T.; Behringer, R.R. Goosecoid is not an essential component of the mouse gastrula organizer but is required for craniofacial and rib development. Development 1995, 121, 3005–3012. [Google Scholar] [CrossRef]
  60. Yamada, G.; Mansouri, A.; Torres, M.; Stuart, E.T.; Blum, M.; Schultz, M.; De Robertis, E.M.; Gruss, P. Targeted mutation of the murine goosecoid gene results in craniofacial defects and neonatal death. Development 1995, 121, 2917–2922. [Google Scholar] [CrossRef]
  61. Gonzalez Malagon, S.G.; Lopez Munoz, A.M.; Doro, D.; Bolger, T.G.; Poon, E.; Tucker, E.R.; Adel Al-Lami, H.; Krause, M.; Phiel, C.J.; Chesler, L.; et al. Glycogen synthase kinase 3 controls migration of the neural crest lineage in mouse and Xenopus. Nat. Commun. 2018, 9, 1126. [Google Scholar] [CrossRef] [PubMed]
  62. Hooper, J.E.; Jones, K.L.; Smith, F.J.; Williams, T.; Li, H. An Alternative Splicing Program for Mouse Craniofacial Development. Front. Physiol. 2020, 11, 1099. [Google Scholar] [CrossRef] [PubMed]
  63. Bain, J.M.; Cho, M.T.; Telegrafi, A.; Wilson, A.; Brooks, S.; Botti, C.; Gowans, G.; Autullo, L.A.; Krishnamurthy, V.; Willing, M.C.; et al. Variants in HNRNPH2 on the X Chromosome Are Associated with a Neurodevelopmental Disorder in Females. Am. J. Hum. Genet. 2016, 99, 728–734. [Google Scholar] [CrossRef] [Green Version]
  64. Marques, F.; Tenney, J.; Duran, I.; Martin, J.; Nevarez, L.; Pogue, R.; Krakow, D.; Cohn, D.H.; Li, B. Altered mRNA Splicing, Chondrocyte Gene Expression and Abnormal Skeletal Development due to SF3B4 Mutations in Rodriguez Acrofacial Dysostosis. PLoS Genet. 2016, 12, e1006307. [Google Scholar] [CrossRef] [Green Version]
  65. Aiello, N.M.; Maddipati, R.; Norgard, R.J.; Balli, D.; Li, J.; Yuan, S.; Yamazoe, T.; Black, T.; Sahmoud, A.; Furth, E.E.; et al. EMT Subtype Influences Epithelial Plasticity and Mode of Cell Migration. Dev. Cell 2018, 45, 681–695.e4. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  66. Cheung, K.J.; Ewald, A.J. A collective route to metastasis: Seeding by tumor cell clusters. Science 2016, 352, 167–169. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  67. Friedl, P.; Locker, J.; Sahai, E.; Segall, J.E. Classifying collective cancer cell invasion. Nat. Cell Biol. 2012, 14, 777–783. [Google Scholar] [CrossRef] [PubMed]
  68. Simeonov, K.P.; Byrns, C.N.; Clark, M.L.; Norgard, R.J.; Martin, B.; Stanger, B.Z.; Shendure, J.; McKenna, A.; Lengner, C.J. Single-cell lineage tracing of metastatic cancer reveals selection of hybrid EMT states. Cancer Cell 2021, 39, 1150–1162.e1159. [Google Scholar] [CrossRef] [PubMed]
  69. Cho, M.S.; Rupaimoole, R.; Choi, H.J.; Noh, K.; Chen, J.; Hu, Q.; Sood, A.K.; Afshar-Kharghan, V. Complement Component 3 Is Regulated by TWIST1 and Mediates Epithelial-Mesenchymal Transition. J. Immunol. 2016, 196, 1412–1418. [Google Scholar] [CrossRef] [Green Version]
  70. Edgar, R.; Domrachev, M.; Lash, A.E. Gene Expression Omnibus: NCBI gene expression and hybridization array data repository. Nucleic Acids Res. 2002, 30, 207–210. [Google Scholar] [CrossRef] [Green Version]
Jdb 11 00029 g001 550
Figure 1. apc is required for the CNC contribution to craniofacial structures: (A) Wild-type (WT) and (B) apcmcr/mcr larvae at ~30 somites (50 hpf). Arrowhead indicates the accumulation of amorphous tissue anterior to the heart and yolk mass. Scale bars in (A,B) are 200 µm. (C,D) Hematoxylin-eosin staining of WT (C) and apcmcr/mcr (D) larvae sectioned at the level of the hindbrain. Hb: hindbrain; S: somite; N: notochord; E: esophagus; L: liver; PF: pectoral fin. Scale bars in (C,D) are 100 µm. (E) Fli1-GFP epifluorescence of WT (top two larvae) and apcmcr/mcr larvae (lower two larvae; 30-somite stage). Arrowheads for WT larvae indicate anterior extent of GFP+ cells in the head, which is reduced or absent in mutants. (F,G) Confocal image of WT; Fli1-GFP (F) and apcmcr/mcr; Fli1-GFP (G) larvae at 60 hpf, showing the vascular endothelium of trunk. (H,I) Confocal image of Fli1-GFP in WT (H) and apcmcr/mcr (I) larvae at 60 hpf, showing CNC and vascular endothelium in branchial arches and head. mc: Meckel’s cartilage; pq: palatoquadrate cartilage; ch: ceratohyal cartilage. Numbers indicate gill arches 1–5.
Figure 1. apc is required for the CNC contribution to craniofacial structures: (A) Wild-type (WT) and (B) apcmcr/mcr larvae at ~30 somites (50 hpf). Arrowhead indicates the accumulation of amorphous tissue anterior to the heart and yolk mass. Scale bars in (A,B) are 200 µm. (C,D) Hematoxylin-eosin staining of WT (C) and apcmcr/mcr (D) larvae sectioned at the level of the hindbrain. Hb: hindbrain; S: somite; N: notochord; E: esophagus; L: liver; PF: pectoral fin. Scale bars in (C,D) are 100 µm. (E) Fli1-GFP epifluorescence of WT (top two larvae) and apcmcr/mcr larvae (lower two larvae; 30-somite stage). Arrowheads for WT larvae indicate anterior extent of GFP+ cells in the head, which is reduced or absent in mutants. (F,G) Confocal image of WT; Fli1-GFP (F) and apcmcr/mcr; Fli1-GFP (G) larvae at 60 hpf, showing the vascular endothelium of trunk. (H,I) Confocal image of Fli1-GFP in WT (H) and apcmcr/mcr (I) larvae at 60 hpf, showing CNC and vascular endothelium in branchial arches and head. mc: Meckel’s cartilage; pq: palatoquadrate cartilage; ch: ceratohyal cartilage. Numbers indicate gill arches 1–5.
Jdb 11 00029 g001
Jdb 11 00029 g002 550
Figure 2. Expression of early and late neural crest markers by in situ hybridization: (A,B) Similar sox10 expression at neural plate border in WT (A) and apcmcr/mcr (B) embryos at 12 hpf. Genotypes in (A) (n = 30 WT or apcmcr/+) and (B) (n = 7 apcmcr/mcr) were defined by genomic PCR on individual larvae. (C,D) In WT embryos at 55 hpf (C), gsc is expressed in the mandibular (m, including Meckel’s cartilage), hyoid (h), and more posterior branchial arches, as well as two symmetric anterior domains, as described previously [44]. In apcmcr/mcr larvae (D), gsc is undetectable in the mandibular and hyoid arches. (For WT, n = 15, and for apcmcr/mcr, n = 7, based on morphological phenotype). All scale bars are 200 µm.
Figure 2. Expression of early and late neural crest markers by in situ hybridization: (A,B) Similar sox10 expression at neural plate border in WT (A) and apcmcr/mcr (B) embryos at 12 hpf. Genotypes in (A) (n = 30 WT or apcmcr/+) and (B) (n = 7 apcmcr/mcr) were defined by genomic PCR on individual larvae. (C,D) In WT embryos at 55 hpf (C), gsc is expressed in the mandibular (m, including Meckel’s cartilage), hyoid (h), and more posterior branchial arches, as well as two symmetric anterior domains, as described previously [44]. In apcmcr/mcr larvae (D), gsc is undetectable in the mandibular and hyoid arches. (For WT, n = 15, and for apcmcr/mcr, n = 7, based on morphological phenotype). All scale bars are 200 µm.
Jdb 11 00029 g002
Jdb 11 00029 g003 550
Figure 3. Transcriptomic analysis of apc loss of function larvae: (A) Heat map showing differential gene expression in WT versus apcmcr/mcr larvae at 48 hpf. To the right is a list of a upregulated genes known to be induced by Wnt/β-catenin activation [45], including multiple Wnt-induced pathway antagonists. (B) RT-qPCR was used to validate changes in expression from RNA-seq data for the indicated mRNAs. GAPDH was used as an input control for RT-qPCR. Error bars show standard error. (C) GO analysis (Metascape [37]) shows the differential expression of genes associated with the indicated terms in apcmcr mutants. (D) Heat map showing the differential expression of mRNAs encoding secreted molecules that regulate neural crest migration and axon guidance. In zebrafish, Complement c3 is encoded by “a” and “b” alleles and the c3a alleles were duplicated to six copies, c3a.1–c3a.6. The “c3a.x” designation for these duplicated genes should be distinguished from the more common designation of the polypeptide “C3a”, the extracellular chemoattractant derived via the proteolytic processing of C3 protein that mediates the co-attraction of CNC cells [11]. The heat map also shows the reduced expression of SDF1/CXCL12 and the differential expression of multiple semaphorins. (E) The abundance of c3a.1, c3a.2, c3a.3, and c3a.6 genes in WT and apcmcr larvae at 48 hpf was based on mean normalized read counts from three independent replicates from RNA-seq data. c3a.5 was excluded because mean read counts were <100 and c3a.4 was not detected. Fold change in expression for apcmcr/WT is shown below graph. Relative change in expression was confirmed for c3a.1 and c3a.6 by RT-qPCR (not shown). Error bars show standard error. ** indicates p < 0.01 (Student’s t-test). (F) GSEA analysis [41] for apcmcr/WT zebrafish identifies parallels with the complement pathway and EMT, as well as c-Myc, canonical Wnt signaling, mTORC1 activation, and inflammatory signaling pathways (Supplemental Table S3).
Figure 3. Transcriptomic analysis of apc loss of function larvae: (A) Heat map showing differential gene expression in WT versus apcmcr/mcr larvae at 48 hpf. To the right is a list of a upregulated genes known to be induced by Wnt/β-catenin activation [45], including multiple Wnt-induced pathway antagonists. (B) RT-qPCR was used to validate changes in expression from RNA-seq data for the indicated mRNAs. GAPDH was used as an input control for RT-qPCR. Error bars show standard error. (C) GO analysis (Metascape [37]) shows the differential expression of genes associated with the indicated terms in apcmcr mutants. (D) Heat map showing the differential expression of mRNAs encoding secreted molecules that regulate neural crest migration and axon guidance. In zebrafish, Complement c3 is encoded by “a” and “b” alleles and the c3a alleles were duplicated to six copies, c3a.1–c3a.6. The “c3a.x” designation for these duplicated genes should be distinguished from the more common designation of the polypeptide “C3a”, the extracellular chemoattractant derived via the proteolytic processing of C3 protein that mediates the co-attraction of CNC cells [11]. The heat map also shows the reduced expression of SDF1/CXCL12 and the differential expression of multiple semaphorins. (E) The abundance of c3a.1, c3a.2, c3a.3, and c3a.6 genes in WT and apcmcr larvae at 48 hpf was based on mean normalized read counts from three independent replicates from RNA-seq data. c3a.5 was excluded because mean read counts were <100 and c3a.4 was not detected. Fold change in expression for apcmcr/WT is shown below graph. Relative change in expression was confirmed for c3a.1 and c3a.6 by RT-qPCR (not shown). Error bars show standard error. ** indicates p < 0.01 (Student’s t-test). (F) GSEA analysis [41] for apcmcr/WT zebrafish identifies parallels with the complement pathway and EMT, as well as c-Myc, canonical Wnt signaling, mTORC1 activation, and inflammatory signaling pathways (Supplemental Table S3).
Jdb 11 00029 g003
Jdb 11 00029 g004a 550Jdb 11 00029 g004b 550
Figure 4. Oncogenic mutations in apc cause widespread splice variations including mRNAs encoding regulators of cell migration: (A) The MAJIQ analysis of splicing variations, represented as changes in fractions spliced in (dPSI) for each splicing event filtered for dPSI ≥ 0.20 with a probability >0.90, identified 340 splicing variations in apcmcr larvae. (B) The frequency of local splice variants, including exon skipping (ES), alternative 3′ splice site (A3SS), alternative 5′ splice site (A5SS), and complex splice variants. (C) The GO analysis of alternative spliced genes. (D) Voila output showing alternative splicing of sema3f (“a” allele). Red line indicates splicing from exon 5 to exon 6 and blue line indicates splicing from exon 5 to exon 7. Violin plots show the frequency of each splice form in WT (left) and apcmcr mutants (right) at 48 hpf. (E). Diagram showing unspliced, nascent mRNA from exon 5–exon 8. Orange arrows indicate PCR primers for “long” splice form that includes exon 6; green arrows show the primer pair for constitutively spliced exons 7 and 8, used to measure all mRNA isoforms. Histogram shows relative abundance based on RT-qPCR for the “long” splice form containing exon 6 in WT and apcmcr mutant larvae at 48 hpf. p < 0.0001 (Student’s paired t-test, n = 3 replicates).
Figure 4. Oncogenic mutations in apc cause widespread splice variations including mRNAs encoding regulators of cell migration: (A) The MAJIQ analysis of splicing variations, represented as changes in fractions spliced in (dPSI) for each splicing event filtered for dPSI ≥ 0.20 with a probability >0.90, identified 340 splicing variations in apcmcr larvae. (B) The frequency of local splice variants, including exon skipping (ES), alternative 3′ splice site (A3SS), alternative 5′ splice site (A5SS), and complex splice variants. (C) The GO analysis of alternative spliced genes. (D) Voila output showing alternative splicing of sema3f (“a” allele). Red line indicates splicing from exon 5 to exon 6 and blue line indicates splicing from exon 5 to exon 7. Violin plots show the frequency of each splice form in WT (left) and apcmcr mutants (right) at 48 hpf. (E). Diagram showing unspliced, nascent mRNA from exon 5–exon 8. Orange arrows indicate PCR primers for “long” splice form that includes exon 6; green arrows show the primer pair for constitutively spliced exons 7 and 8, used to measure all mRNA isoforms. Histogram shows relative abundance based on RT-qPCR for the “long” splice form containing exon 6 in WT and apcmcr mutant larvae at 48 hpf. p < 0.0001 (Student’s paired t-test, n = 3 replicates).
Jdb 11 00029 g004aJdb 11 00029 g004b
Table
Table 1. Primers for reverse transcription-quantitative PCR (RT-qPCR).
Table 1. Primers for reverse transcription-quantitative PCR (RT-qPCR).
RT-qPCRForwardReverse
CCL19 CCCCATTGCAGCTACTGTATTC AGGTGTTTTTCTCTGGTGGGG
IL-11aCCGGTTCAAGTCTCTTCCAGAGGTTTGCATGGAGCTGAGA
IL-11bCATCTTATCCAAGCTATCATCCAGGATCTCGGGTGCTGTCTGTC
LEPA GGAACACATTGACGGGCAAA ATGGGTTTGTCAGCGGGAAT
CBX7a TGCGGTGGAGTCAATAACGAA CAGGTGCTGTACTTAGGCGA
DKK1a GTGGAGTTTGTCTGTCGTGC AAGCTGACACACACCGTTGA
DKK1b CACCGCAGCAGCCTTTAATC CGCGAGACTGGAAGCAAAAC
NOTUM1a CACCTGTAACGACGGGACTC CCAGCCGCCCTCAAGAAATA
LFT1 ACGCACGAGTGAGCATCTAC CGTGAATGGGAATCAACCTGG
SALL1b CTTCAGGGAGATAACCCGGC CCATCGTATGATCGAGGAGAACA
SOCS3a AAGCAGGGAAGACAAGAGCC AGAGCTGGTCAAAAGAGCCTAT
GSC CCTACAGGTTATGACAGCGCC GACAAGGTGCCCACGTTCAT
EMILIN3a GGCACAAGAACCACTGTGCAT CCAAGCACACTTCATTGCCT
GAPDH GTGGAGTCTACTGGTGTCTTC GTGCAGGAGGCATTGCTTACA
C3A.1 GACGCCCAACTTGAAACCAC GCAACCTCAGGGATGGCATA
C3A.6 ACCAGGAATGCCCTTCAGTG ACCTTTGACTCCTCCGGGAT
RT-qPCR for splice forms:
SEMA3fa_ALL ACTCAACAGCGTCTCAGCTT TACTGGTCGGTCCTCATTGC
SEMA3fa_Long splice form ACAACCCCATCTGCACCTATG TCTGGTGAGGCACTAGGGT
Disclaimer/Publisher’s Note: The statements, opinions and data contained in all publications are solely those of the individual author(s) and contributor(s) and not of MDPI and/or the editor(s). MDPI and/or the editor(s) disclaim responsibility for any injury to people or property resulting from any ideas, methods, instructions or products referred to in the content.

Share and Cite

MDPI and ACS Style

Liu, X.; Jones, W.D.; Quesnel-Vallières, M.; Devadiga, S.A.; Lorent, K.; Valvezan, A.J.; Myers, R.L.; Li, N.; Lengner, C.J.; Barash, Y.; et al. The Tumor Suppressor Adenomatous Polyposis Coli (apc) Is Required for Neural Crest-Dependent Craniofacial Development in Zebrafish. J. Dev. Biol. 2023, 11, 29. https://doi.org/10.3390/jdb11030029

AMA Style

Liu X, Jones WD, Quesnel-Vallières M, Devadiga SA, Lorent K, Valvezan AJ, Myers RL, Li N, Lengner CJ, Barash Y, et al. The Tumor Suppressor Adenomatous Polyposis Coli (apc) Is Required for Neural Crest-Dependent Craniofacial Development in Zebrafish. Journal of Developmental Biology. 2023; 11(3):29. https://doi.org/10.3390/jdb11030029

Chicago/Turabian Style

Liu, Xiaolei, William D. Jones, Mathieu Quesnel-Vallières, Sudhish A. Devadiga, Kristin Lorent, Alexander J. Valvezan, Rebecca L. Myers, Ning Li, Christopher J. Lengner, Yoseph Barash, and et al. 2023. "The Tumor Suppressor Adenomatous Polyposis Coli (apc) Is Required for Neural Crest-Dependent Craniofacial Development in Zebrafish" Journal of Developmental Biology 11, no. 3: 29. https://doi.org/10.3390/jdb11030029

Note that from the first issue of 2016, this journal uses article numbers instead of page numbers. See further details here.

Article Metrics

Back to TopTop