The novel ciliogenesis regulator DYRK2 governs Hedgehog signaling during mouse embryogenesis
Abstract
Mammalian Hedgehog (Hh) signaling plays key roles in embryogenesis and uniquely requires primary cilia. Functional analyses of several ciliogenesis-related genes led to the discovery of the developmental diseases known as ciliopathies. Hence, identification of mammalian factors that regulate ciliogenesis can provide insight into the molecular mechanisms of embryogenesis and ciliopathy. Here, we demonstrate that DYRK2 acts as a novel mammalian ciliogenesis-related protein kinase. Loss of Dyrk2 in mice causes suppression of Hh signaling and results in skeletal abnormalities during in vivo embryogenesis. Deletion of Dyrk2 induces abnormal ciliary morphology and trafficking of Hh pathway components. Mechanistically, transcriptome analyses demonstrate down-regulation of Aurka and other disassembly genes following Dyrk2 deletion. Taken together, the present study demonstrates for the first time that DYRK2 controls ciliogenesis and is necessary for Hh signaling during mammalian development.
Introduction
Embryogenesis and patterning of cell differentiation are facilitated by spatiotemporal activation of multiple signaling pathways. The Hedgehog (Hh) signaling is an evolutionarily conserved system that plays a central role in embryogenesis via regulating cell proliferation and differentiation (Ingham and McMahon, 2001). Upon stimulation by ligands, post-translational modification of GLI2 and GLI3 induces the expression of Gli1, which is a key amplifier of Hh signaling. These post-translational and transcriptional activations of three GLIs regulate specific and redundant target genes (Mo et al., 1997; Hui and Angers, 2011). Hence, mutants of Hh components cause typical defects such as skeletal, neural, and retinal abnormalities (Mo et al., 1997).
Unlike other core developmental signaling, vertebrate Hh signaling is uniquely and completely dependent upon primary cilia, which are microtubule-based organelles that are formed during the G0 or G1 phases of the cell cycle (Huangfu et al., 2003). Binding of Hh ligands to Patched 1 (PTCH1) on cilia leads to activation and induction of Seven-spanner smoothened (SMO) to the cilia (Rohatgi et al., 2007). Activated SMO leads to recruitment of GLI2 and GLI3 to the cilia tip via inhibition of protein kinase A (Chen et al., 2009; Kim et al., 2009; Wen et al., 2010). This dynamic ciliary trafficking of Hh components is primarily regulated by intraflagellar transport (IFT) (Haycraft et al., 2005; Eguether et al., 2014). Thus, ciliogenesis is indispensable for tissue development, and defects in this process impact the development of multiple organs to cause human and mouse diseases termed ‘ciliopathies’ (Reiter and Leroux, 2017). Accordingly, the typical phenotype observed in some of ciliopathies such as Joubert syndrome is abnormalities of Hh signaling (Bangs and Anderson, 2017).
Mutations in a number of different ciliopathy-associated genes often result in alterations of ciliary length (Paige Taylor et al., 2016; Reiter and Leroux, 2017). Indeed, genetic screenings of Chlamydomonas, which is a model organism for ciliogenesis, have identified the ciliopathy-associated genes controlling cilia length to generate the optimal length at steady-state (Wemmer and Marshall, 2007). Although these abnormalities in ciliary length are thought to be controlled by the balance of assembly and disassembly via IFT and a postulated length sensor, the mechanisms for maintaining the cell-type-specific ciliary length have not been fully elucidated (Ishikawa and Marshall, 2011). In contrast, the ciliary resorption mechanisms for cell cycle re-entry have been thoroughly investigated by such as an experiment of serum re-addition to starved cells, and these mechanisms include the HEF1-AURKA-HDAC6 pathway (Pugacheva et al., 2007), the PLK-KIF2A pathway (Wang et al., 2013), and the NEK2-KIF24 pathway (Kobayashi et al., 2011; Kim et al., 2015b) that have been observed to induce disassembly of cilia. On the other hand, the ability of these ciliary resorption factors for cell cycle re-entry to control cilia length at steady-state and during ciliogenesis remains to be elucidated. Hence, identification of novel mammalian factors regulating ciliogenesis and ciliary length control will provide insight into the molecular mechanisms underlying embryogenesis and ciliopathy as well as ciliary functions.
Dual-specificity tyrosine-regulated kinase (DYRK) is a family that belongs to the CMGC group that includes cyclin-dependent kinases (CDK), mitogen-activated protein kinase (MAPK), glycogen synthase kinase (GSK), and CDK-like kinase (CLKs) (Becker and Sippl, 2011). Two isoforms of Dyrk2 have been identified; long and short forms, the latter lacks a 5’ terminal region. In human cancer cells, we have functionally identified DYRK2 as a regulator of p53-induced apoptosis in response to DNA damage (Taira et al., 2007) and of G1/S transition (Taira et al., 2012). During development in lower eukaryotes, MBK2, which is an ortholog of DYRK2 in Caenorhabditis elegans, regulates maternal-protein degradation during the oocyte-to-embryo transition via a ubiquitin-dependent mechanism (Pellettieri et al., 2003; Pang et al., 2004; Lu and Mains, 2007; Yoshida and Yoshida, 2019). While these reports lead us to speculate that DYRK2 must also play important roles in mammalian development, no reports are available regarding the mechanistic role of DYRK2 in vivo.
In the present study, we aim to reveal a function for DYRK2 in mammalian development in vivo. Here, we demonstrate that DYRK2 is a novel regulator of ciliogenesis and is required for normal embryogenesis via activation of Hh signaling during development.
Results
Dyrk2 deficiency cause suppression of Hedgehog signaling during mouse embryogenesis
We generated Dyrk2 knockout mice (Dyrk2-/-) by eliminating the third exon of the Dyrk2 genomic locus (Figure 1—figure supplement 1A–B). The absence of DYRK2 protein in homozygous Dyrk2-/- mice was confirmed (Figure 1—figure supplement 1C). Although the gross morphology of homozygous Dyrk2-/- embryos appeared normal during early development, multiple defects became obvious during later stages of gestation, and the mice died at or close to birth (Figure 1A). Specifically, defects in skeletal development were remarkable, and these included a shorter dorsum of the nose (Figure 1A), cleft palate including hypoplasia of the tongue (Figure 1B–C), loss of the basisphenoid, basioccipital, and presphenoid bones (Figure 1D), shorter limbs (Figure 1E), defects of segmentation of the sternebrae in the sternum (Figure 1F), and vertebra (Figure 1G) at embryonic day (E) 18.5. These skeletal defects that included reduction of bone mineralization were observed until E16.5 (Figure 1H).
As Dyrk2-/- embryos at E18.5 exhibited a similar phenotype to that observed in response to certain defects in Hh signaling (Mo et al., 1997), we assessed Gli1-expression, which is an indicator of Hh signaling activation (Niewiadomski and Rohatgi, 2015). In situ hybridization demonstrated that Gli1-expression was decreased in the craniofacial region in Dyrk2-/- embryos at E14.5 (Figure 2A). Protein levels of GLI1 were also decreased at E13.5 (Figure 2B). Ptch1-expression, which is another indicator of Hh signaling activation (Snouffer et al., 2017), was also decreased in Dyrk2-/- embryos at E13.5, and this was accompanied by a decrease in Gli1; however, Shh-expression remained unchanged (Figure 2C). We also observed a repression of Foxf2-expression, which is a direct target gene of GLI1 (Everson et al., 2017), in the craniofacial region of Dyrk2-/- embryos (Figure 2D–E).
Loss of genes required for Hh signaling often causes defects in dorsal-ventral neural tube patterning, which is regulated by the SHH morphogen (Dessaud et al., 2008). Although we investigated the localization patterns of FOXA2, NKX2.2, OLIG2, NKX6.1, and PAX6 at E10.5, we did not observe obvious differences in their expression patterns (Figure 2—figure supplement 1A). Expression of Hh target genes was decreased in Dyrk2-/- whole embryos at E9.5 (Figure 2—figure supplement 1B). In situ hybridization demonstrated that Ptch1-expression was decreased in the mandibular arch in Dyrk2-/- embryos at E10.5, but remained unchanged in the neural tube (Figure 2—figure supplement 1C). These data showing the maintenance of Hh signal and dorsal-ventral patterning in the neural tube might correspond to a spatiotemporal expression-pattern of Dyrk2.
Taken together, Dyrk2-deficient embryos exhibit a robust suppression of Hh signaling and possess particular skeletal abnormalities during embryogenesis.
DYRK2 positively regulates Hh signaling
To investigate the defect in Hh signaling in Dyrk2-/- mice in more detail, we analyzed primary mouse embryonic fibroblasts (MEFs) derived from wild-type and Dyrk2-/- mice. First, we measured Hh signaling activity in response to stimulation with the SMO agonist SAG. In response to stimulation with SAG, Gli1 and Ptch1 expression was increased in wild-type mice as previously reported (Figure 3A; Niewiadomski and Rohatgi, 2015). In contrast, in Dyrk2-/- MEFs, inductions of both Gli1 and Ptch1 expression by SAG was drastically repressed (Figure 3A). Consistent with gene expression analyses, the induction of GLI1 protein by SAG stimulation was also suppressed in Dyrk2-/- MEFs (Figure 3B). Immunocytostaining for GLI1 following stimulation with SAG demonstrated that the accumulation of GLI1 protein within nuclei was clearly diminished in Dyrk2-/- MEFs (Figure 3C). To validate whether these phenotypes observed in Dyrk2-/- MEFs are due to abnormal differentiation caused by deletion of Dyrk2 during early embryogenesis, we performed a transient knockdown of Dyrk2 in wild-type MEFs using two independent short interfering RNAs (siRNAs). Transient knockdown of Dyrk2 also demonstrated suppression of both the mRNA and protein levels of Gli1 and Ptch1 in response to stimulation with SAG (Figure 3—figure supplement 1A–B).
To validate this suppression of Hh signaling by Dyrk2-deletion, we performed a transient over-expression experiment using wild-type human DYRK2 or a DYRK2-K251R construct that expresses a kinase dead mutant (Taira et al., 2012; Figure 3—figure supplement 1C–D) in Dyrk2-/- MEFs using adenovirus infection (Yokoyama-Mashima et al., 2019). Over-expression of the wild-type DYRK2 construct restored significant induction of Gli1 and Ptch1 expression upon exposure to SAG (Figure 3D, Figure 3—figure supplement 1D). In sharp contrast, over-expression of the DYRK2-K251R construct in Dyrk2-/- MEFs markedly diminished Gli1 and Ptch1 expression (Figure 3D). Additionally, over-expression of the DYRK2-K251R construct slightly increased Gli1 and Ptch1 expression in comparison with that of empty vector (Figure 3D). This kinase-independent effect might be associated with a function of DYRK2 as a scaffold protein (Maddika and Chen, 2009). Taken together, the induction of Hh signaling is drastically suppressed by deletion of Dyrk2 in a kinase activity-dependent manner.
The key Hh pathway components GLI2 and GLI3 are known to be posttranslationally modified in a manner that is dependent upon Hh ligands (Mo et al., 1997; Hui and Angers, 2011). In the absence of Hh ligands, the full-length proteins (active forms; GLI2 and GLI3FL) are phosphorylated by multiple kinases, leading to proteasomal degradation or truncation into N-terminal repressor forms (GLI3REP), respectively (Niewiadomski and Rohatgi, 2015). In this context, we analyzed the endogenous protein levels and states of GLI2 and GLI3. In wild-type MEFs, immunoblotting for GLI2 revealed that full-length form of GLI2 was increased by SAG-stimulation (Figure 3E–F). In contrast to wild-type MEFs, the increase of GLI2 protein levels by SAG was significantly suppressed in Dyrk2-/- MEFs (Figure 3E–F). We also analyzed two forms of GLI3 (GLI3FL and GLI3REP). SAG-stimulation suppressed the formation of GLI3REP and decreased the ratio of GLI3REP/GLI3FL in wild-type MEFs (Figure 3—figure supplement 2; Niewiadomski and Rohatgi, 2015). In Dyrk2-/- MEFs, however, we found that the ratio of GLI3REP/GLI3FL was marginally suppressed and that no significant differences between the absence or presence of SAG existed (Figure 3—figure supplement 2D). Collectively, these data indicate that the deletion of Dyrk2 affects the stabilities of GLI2, and marginally GLI3, under SAG-stimulation.
DYRK2 regulates ciliogenesis
As primary cilia are essential organelles required for signal transduction of vertebrate Hh signaling (Huangfu et al., 2003), we investigated whether DYRK2 regulates ciliogenesis in MEFs. Immunostaining of acetylated tubulin (a cilia axoneme marker) and γ-tubulin (a basal body marker) demonstrated that the length of primary cilia in Dyrk2-/- MEFs was significantly longer than that in wild-type MEFs (Figure 4A). The average cilia length in wild-type MEFs was 1.65 ± 0.03, while it was 3.59 ± 0.08 in Dyrk2-/- MEFs (Figure 4B–C). In addition to the increased length, the morphology of primary cilia in Dyrk2-/- MEFs was often bulged at the tips, tapered, and twisted (Figure 4A). This elongation and morphological abnormality of primary cilia was similarly observed in response to the transient knockdown of Dyrk2 by siRNA in wild-type MEFs (Figure 4—figure supplement 1). To investigate whether the regulation of ciliogenesis by DYRK2 is conserved in other species and cell types, we analyzed immortalized human retinal pigment epithelia cells (hTERT-RPE1 cells) that are commonly used to study cilia-assembly and -disassembly. A transient knockdown by siDYRK2 also induced a significant elongation and morphological abnormality in cilia of these cells (Figure 4—figure supplement 2). In contrast to the length and morphology of primary cilia, no difference was observed on the proportion of ciliated cells in wild-type and Dyrk2-/- MEFs (Figure 4—figure supplement 3A–B). Similarly, in cell-cycling (KI67-positive) wild-type and Dyrk2-/- MEFs, there was comparable in the proportion of ciliated cells (ciliated cells in KI67-positive cells is 1 per 199 and 1 per 139 cells in wild-type and Dyrk2-/- MEFs, respectively) (Figure 4—figure supplement 3C).
To confirm the morphological abnormalities of primary cilia within the tissue, we performed scanning electron microscopy (SEM) on embryos at E10.5. SEM images clearly showed that the cilia of Dyrk2-/- embryos were significantly elongated, bulged at the tips, and twisted, while those of wild-type embryos were shortened and straight (Figure 4D). These abnormalities were also observed in several types of cells, including mesenchymal cells (Figure 4E), chondrocytes, neuroepithelium, and tongue cells (data not shown) in the embryonic craniofacial region at E13.5 as assessed by immunohistochemistry.
These data indicating that deletion of Dyrk2 causes morphological abnormalities in primary cilia prompted us to determine the subcellular localization of DYRK2. We transfected DYRK2-HaloTag constructs into hTERT-RPE1 cells and induced ciliogenesis by serum-starvation. Immunocytostaining for both anti-HaloTag and anti-DYRK2 revealed that DYRK2 localized at γ-tubulin-positive basal bodies and at the proximal end of the axoneme, namely a transition zone (TZ) (Figure 5A–B). No signal for anti-HaloTag (Figure 5C) or anti-DYRK2 (data not shown) was observed in hTERT-RPE1 cells transfected with empty vector (pFN22K-Halo Tag-CMVd1-Flexi-vector). Moreover, immuno-positive signals for DYRK2-HaloTag were co-localized with a TZ marker, NPHP1 (Figure 5D).
These data indicated that DYRK2 might regulate ciliogenesis at basal bodies and TZ in vivo and in vitro.
Deletion of DYRK2 induces abnormal ciliary trafficking of Hedgehog pathway components
In mammals, key regulators of Hh signaling have been demonstrated to be recruited and activated at the cilia upon Hh stimulation (Chen et al., 2009; Kim et al., 2009; Tukachinsky et al., 2010; Wen et al., 2010), and disorders in the ciliary trafficking of Hh components cause dysfunction of Hh signaling (He et al., 2014). To investigate whether inactivation of Hh signaling in Dyrk2-/- embryos and MEFs is due to abnormal ciliary trafficking of Hh components, we analyzed the ciliary localization of key regulators such as SMO, GLI2, GLI3, and SuFu. In wild-type MEFs, immuno-positive SMO signals were mostly undetectable or faint in the absence of Hh stimulation, and recruitment to cilia was dependent upon Hh stimulation (Figure 6A–B), as shown in a previous report (Tukachinsky et al., 2010). Similarly, no significant difference in the frequency of SMO recruitment in response to SAG stimulation was observed in Dyrk2-/- MEFs (Figure 6A–B).
We subsequently analyzed the ciliary localization of endogenous GLI2 and GLI3. As shown in a previous report (Tukachinsky et al., 2010), in wild-type MEFs, immuno-positive signals for both GLI2 and GLI3 were mostly undetectable or faint in the absence of Hh stimulation, and SAG stimulation increased the presence of GLI2 and GLI3 at cilia tips (Figure 6C–F). In contrast, in Dyrk2-/- MEFs, immuno-positive signals for both GLI2 (approximately 75.9% of cilia) and GLI3 (approximately 95.8%) were observed at cilia tip even in the absence of SAG treatment (Figure 6C–F). Moreover, the intensity of immune-positive signals was markedly increased by SAG-treatment in Dyrk2-/- MEFs (Figure 6C,E). These accumulations at cilia tips were frequently observed in Dyrk2-/- mesenchymal cells in the craniofacial region at E10.5 tissues but were absent in wild-type cells (Figure 6—figure supplement 1). Additionally, localization of SuFu, which forms a complex with both GLI2 and GLI3 (Tukachinsky et al., 2010), was disordered in cilia tips in a similar pattern to that of GLI2 and GLI3 (Figure 6—figure supplement 2A). Collectively, ciliary localization of GLI2, GLI3, and SuFu in Dyrk2-/- MEFs and embryos was clearly disordered and was accumulated at cilia tips. Importantly, the recruitment of GLI2, GLI3, and SuFu in response to SAG stimulation was also observed in Dyrk2-/- MEFs.
Inhibition of retrograde transport from the tip to the cell body induces accumulation of Hh components and results in abnormal localization of both IFT-A (implicated in retrograde IFT) and IFT-B (implicated in anterograde) (Ocbina and Anderson, 2008; Ocbina et al., 2011; Liem et al., 2012). Based on this, we analyzed the ciliary localization of core IFT-A (IFT140) and IFT-B (IFT81 and IFT88) (Nakayama and Katoh, 2018). In Dyrk2-/- MEFs, no obvious differences in ciliary localization of IFT140, IFT81, and IFT88 were observed (Figure 6—figure supplement 2B–D).
Activation of mammalian target of rapamycin complex 1 (mTORC1) also induces abnormal trafficking and elongates cilia length (Broekhuis et al., 2014). mTORC1 activation leads to phosphorylation of ribosomal S6 kinase (S6K) and eukaryotic translational initiation factor 4E binding protein (4EBP). In Dyrk2-/- MEFs, phosphorylation of both S6K and 4EBP was slightly increased (Figure 6—figure supplement 3A); however, treatment with rapamycin, an inhibitor of mTORC1, resulted in no obvious differences in cilia length in Dyrk2-/- MEFs (Figure 6—figure supplement 3B–D).
Moreover, a centrosome protein CP110 (Hossain et al., 2017) and a microtubule severing enzyme, KATANIN p60 (Maddika and Chen, 2009), have been identified as substrates of DYRK2 for proteolysis. In Dyrk2-/- MEFs, however, no obvious difference in protein levels of both CP110 and KATANIN p60 was observed (Figure 6—figure supplement 4).
Deletion of Dyrk2 dysregulates the expression of Aurka and other cilia-disassembly genes
To understand the molecular mechanisms underlying cilia dysfunction in Dyrk2-/- mice, we focused on factors that are involved in ciliary length control by incorporating whole-genome RNA sequencing using wild-type and Dyrk2-/- MEFs (Figure 7, Figure 7—figure supplement 1). The data were analyzed by multiple testing and according to p-value, false discovery rate (FDR), and ratio (Dyrk2-/-/wild-type). As a result, the number of identified genes was 53 or 42 that were significantly downregulated (p<0.005, ratio <1.5 fold) or upregulated (p<0.005, ratio >1.5 fold) in Dyrk2-/- MEFs, respectively, regardless of the presence or absence of SAG (Table 1). Notably, GO and STRING analysis revealed that the 53 downregulated genes in Dyrk2-/- MEFs were enriched in cell division (GO: 0051301, FDR = 5.17E-40), microtubule cytoskeleton organization (GO:0000226, FDR = 5.23E-15), spindle organization (GO:0007051, FDR = 2.72E-11), mitotic cell cycle checkpoint (GO:0007093, FDR = 3.78E-07), and microtubule-based movement (GO:0007018, FDR = 3.9E-4) (Figure 7A, Figure 7—figure supplement 1B). These downregulated genes in Dyrk2-/- MEFs included those related to ciliary resorption mechanisms for proliferation, including the HEF1-AURKA-HDAC6 pathway (Aurka, Plk1, Ube2c, and Tpx2) (Pugacheva et al., 2007), the PLK-KIF2A pathway (Plk1 and Kif2c, a family of Kif2a) (Wang et al., 2013), and the APCCDC20-Nek1 pathway (Cdc20) that controls ciliary length (Wang et al., 2014; Keeling et al., 2016). We confirmed the downregulation of Aurka, Plk1, Ube2c, Tpx2, Kif2c, and Cdc20 in Dyrk2-/- MEFs by qPCR (Figure 7B). To identify a molecule involved in cilia-elongation in Dyrk2-/- cells, we performed transient knockdown of selected genes using siRNA in wild-type MEFs, and we analyzed cilia length. Notably, we found that knockdown of Aurka by two independent siRNAs significantly increases cilia length (Figure 8). Moreover, we performed a rescue experiment by over-expression of AURKA-EGFP in Dyrk2-/- MEFs (Figure 9). Immunostaining and measurement of the cilia length in EGFP- (transfected with pEGFP-C1) or AURKA-EGFP-positive (transfected with Aurka/pEGFP-C1) Dyrk2-/- MEFs demonstrated that elongated cilia in Dyrk2-/- MEFs were significantly shortened in AURKA-EGFP-positive cells in comparison with EGFP-positive ones (Figure 9D–G).
These findings collectively support the potential mechanism that DYRK2 governs ciliogenesis by, at least in part, maintaining the expression of Aurka and other disassembly genes.
Discussion
DYRK2 is a positive regulator of Hh signaling
Although evidence indicates that DYRK2 plays important roles in the development of lower eukaryotes (Pellettieri et al., 2003; Pang et al., 2004; Lu and Mains, 2007), little is known regarding the functions of DYRK2 in mammalian development. In the present study, we demonstrate for the first time that DYRK2 is required for normal Hh signaling and embryogenesis in vivo. Varjosalo et al. have established a human full-length protein kinase cDNA and corresponding kinase activity-deficient mutant library, and they reported that DYRK2 functions as a negative regulator of Hh signaling via direct phosphorylation and induction of the proteasome-dependent degradation of GLIs using in vitro over-expression approaches (Varjosalo et al., 2008). In sharp contrast, our present study demonstrated using knockout approaches that endogenous protein levels of GLI2, and marginally the ratio of GLI3REP/GLI3FL, are decreased by deletion of Dyrk2 in vitro after SAG-treatment. Consistently, Dyrk2-/- embryos exhibited some typical phenotypes of inactivation of Hh signaling in vivo as indicated by abnormal responses but not the elimination of ligands. Taken together with the observed loss of Gli1 induction in Dyrk2-/- MEFs in vitro, we concluded that DYRK2 functions as a positive regulator of Hh signaling. GLI2 and GLI3, the key mediators of Hh signaling, are known to have specific and redundant functions (Mo et al., 1997). In skeletal patterning during development, Dyrk2-/- embryos exhibit phenotypes that are more similar to those of double Gli2 and Gli3 mutants than to those of each single mutant. Conversely, the deletion of other indispensable upstream Hh components such as Smo (Norman et al., 2009), Ptch1 (Svärd et al., 2006), Gpr161 (Hwang et al., 2018), and SuFu (Svärd et al., 2006) results in more severe defects that occur at earlier embryonic stages. The present data do not rule out the possibility that DYRK2 directly regulates Hh components. Despite this, given the evidence that Dyrk2-/- embryos and cells possess morphological abnormalities in primary cilia, it is clear that DYRK2 plays a pivotal role in regulating Hh signaling via the control of ciliogenesis.
Dyrk2 is a novel ciliogenesis-related gene in mice
Intriguingly, we found that DYRK2 negatively regulates ciliogenesis. In Chlamydomonas, certain mutations that cause flagella to assemble to excessive length (i.e. negatively regulator of ciliogenesis) have been identified, and these include mutations in LF1 through LF5 (Wilson et al., 2008; Tam et al., 2013). Among these, LF2, LF4, and LF5 encode protein kinases and are homologs of vertebrate CCRK, MAK/ICK/MOK, and CDKL5, respectively. In addition to these genes, GSK3β also negatively regulates cilia and flagella length (Yuan et al., 2012). Interestingly, DYRK2 belongs to the same kinase group as CCRK, MAK/ICK/MOK, CDKL5, and GSK3β (the CMGC group) (Becker and Sippl, 2011). To the best of our knowledge, however, the present study demonstrates for the first time that DYRK2 is a ciliogenesis-related gene and a negative regulator of ciliogenesis. Among these kinases, Dyrk2-/- embryos exhibit similar phenotypes to Ick-deletion mice in vivo such as skeletal defects and cilia morphology, although they do not possess a hydrocephalus defect (Moon et al., 2014). In response to Ick- or Mok-knockdown, cilia length depends on the activation of mTORC1 signaling (Bolton et al., 2007). Our previous study reported the activation of mTORC1 signaling in DYRK2-knockdown human breast cancer cells (Mimoto et al., 2017). As expected, mTORC1 signaling was slightly activated in Dyrk2-/- MEFs; however, rapamycin, an inhibitor of mTORC1, did not significantly affect cilia length in Dyrk2-/- MEFs. Thus, DYRK2 may control ciliogenesis through different mechanisms than those of other CMGC-kinases.
DYRK2 is required for ciliogenesis and the dynamic trafficking of Hedgehog components in cilia
Abnormal ciliary trafficking of Hh components causes dysfunction in Hh signaling in several types of mutant mice (He et al., 2014; Moon et al., 2014). Dyrk2-/- MEFs and embryos possessed disordered accumulation of Hh components (GLI2, GLI3, and SuFu) at cilia tips and exhibited elongation of cilia. On the other hand, SMO recruitment dependent on ligand stimulation was normally observed in Dyrk2-/- MEFs (Figure 10). Moreover, DYRK2 localizes at TZ, which acts as a selective barrier to control ciliary import and export of proteins (Gerhardt et al., 2016). Given the findings that ciliary localization and ciliary disorders were observed in Dyrk2-/- cells, DYRK2 could be involved in regulation of ciliary protein entry and exit. The functions of DYRK2 at TZ, however, remains to be elucidated.
As a first step to elucidate the functions of DYRK2 in cilia, we focused on factors involved in ciliary length control using a transcriptome approach, and we identified the downregulation of genes related to ciliary resorption mechanisms for proliferation in Dyrk2-/- MEFs, such as Aurka, Plk1, Ube2c, Tpx2, Kif2c, and Cdc20. Among these, AURKA has been well-characterized as a disassembly factor, as transient knockdown by siRNA or treatment with an inhibitor of AURKA completely blocked ciliary disassembly during proliferation (Pugacheva et al., 2007; Inoko et al., 2012). In contrast to ciliary disassembly under proliferation, the function of AURKA for controlling ciliary length at steady state is unclear. In the present study, transient knockdown of Aurka under serum-starvation conditions induced elongation of cilia in a manner similar to that observed in Dyrk2-/- MEFs. These data imply that the down-regulation of Aurka is, at least in part, associated with the phenotypes observed after deletion of Dyrk2. The expression of Aurka is known to be regulated by pathways such as YAP/TAZ (Kim et al., 2015a) and AKT signaling (Plotnikova et al., 2015). The molecular mechanisms underlying DYRK2-mediated Aurka regulation and ciliary trafficking remain unclear. Further research is required to elucidate these mechanisms.
A possible relationship between DYRK2 and human ciliopathy
A number of syndromes caused by disorders involving ciliary proteins are categorized as skeletal ciliopathies, and these include short-rib thoracic dysplasia (SRTD), Jeune asphyxiating thoracic dystrophy (JATD), orofaciodigital syndrome (OFD), Ellis-van Creveld syndrome (EVC), and cranioectodermal dysplasia (CED) (Reiter and Leroux, 2017). In mice, deletion of Dyrk2 induces morphological abnormalities in primary cilia and skeletal defects in vivo. Additionally, DYRK2 is a ciliary protein that is primarily localized at the basal body and the TZ, which contains a growing number of ciliopathy proteins (Reiter et al., 2012). While the present study does not include any evidence to support the relationship between DYRK2 and human disease, our results do suggest a possibility that DYRK2 is involved in human ciliopathy, particularly in regard to skeletal disorders. Further investigations involving exome sequencing or genome-wide association studies using human patients will prove useful to clarify this issue.
Conclusion
In summary, we identified DYRK2 as a novel mammalian ciliogenesis-related gene in vivo and in vitro. Deletion of Dyrk2 induces abnormal ciliary morphology and trafficking of Hh pathway components and suppresses Hh signaling during mouse embryogenesis. The abnormal ciliogenesis in Dyrk2-/- cells is partially caused by downregulation of Aurka and other disassembly genes. These findings will allow for a more complete understanding of the molecular mechanisms underlying embryogenesis, ciliogenesis, and human ciliopathy.
Materials and methods
Generation of Dyrk2 knockout mice (Dyrk2-/-)
Request a detailed protocolDyrk2-/- mice were generated using the knockout-first strategy (Skarnes et al., 2011). A schematic representation of the targeted Dyrk2 allele is provided in Figure 1—figure supplement 1A. The Dyrk2 targeting vector (PG00105_X_1_G09 and PG00105_X_1_E04) was obtained from the Knockout Mouse Project Repository (Dyrk2 targeting project: 337–66440). Gene-targeting methods were performed according to standard protocols. Briefly, linearized vectors were electroporated into JM8A3.N1 embryonic stem (ES) cells. G418-resistant ES cell clones were analyzed using Southern blot analysis for the presence of the correct targeted-allele using BglII digestion and a 3’ external probe. Hybridization with the 3’ external probe detected 10.7 kb (wild-type allele) and 17.0 kb (targeted tm1a allele) BglII bands (Figure 1—figure supplement 1A). Six positive ES clones out of 240 clones were obtained. Chimeric mice were created by injection of the targeted ES cells into C57BL/6J blastocysts and were mated with C57BL/6J WT mice to establish germline-transmitted founders. Heterozygous knockout-first (Dyrk2tm1a) mice were identified using Southern blotting. An exon three knockout allele (Dyrk2tm1b) was generated by mating the Dyrk2tm1a mice the with CAG-Cre mice (Figure 1—figure supplement 1A). For genotyping and validation of knockout alleles, we performed PCR using the primers listed in Table 2.
Animal care
Request a detailed protocolMice were housed individually in a temperature-controlled room under a 12 hr light/dark cycle. Determination of pregnancy in mice was achieved by the observation of a vaginal plug on day 0.5 of gestation. Animals were euthanized by anesthesia. The animal experiment protocol was approved by the Institutional Animal Care and Use Committee of Jikei University (No. 2017–065 and 2018–031), and the studies were performed in accordance with the Guidelines for the Proper Conduct of Animal Experiments of the Science Council of Japan.
Alcian blue and alizarin red staining
Request a detailed protocolEuthanized wild-type and Dyrk2-/- mice at E18.5 and E16.5 were skinned, eviscerated, and fixed in 100% EtOH. For skeletal analysis, the embryos were stained with 1% Alcian Blue (Wako Pure Chemicals, Osaka, Japan) dissolved in 20% glacial acetic acid and 80% EtOH and 0.01% Alizarin Red (Sigma-Aldrich, St. Louis, MO) dissolved in 1% KOH. The excised tissues were observed using a stereo microscope (BioTools, Gunma, Japan). Ten embryos of each wild-type and Dyrk2-/- mice were analyzed.
In situ hybridization
Request a detailed protocolIn situ hybridization was performed according to a previous report (Fujiwara et al., 2007). Briefly, each digoxigenin (DIG)-labeled cRNA probe was amplified by PCR using primer sets (Table 2) and labeled using the Roche DIG RNA labeling kit (Merck, Schwalbach, Germany). Embryos at E10.5 and the heads of mice at E14.5 were fixed using MEMFA (2 mM EGTA, 1 mM MgSO4, and 3.7% formaldehyde) in 100 mM MOPS (pH 7.5) overnight at 4°C, and this was followed by immersion in 30% trehalose (Wako) in 20 mM HEPES to cryoprotect the tissues. Cryosections (7 μm thickness) from the transverse or sagittal plane were hybridized with DIG-labeled cRNA probe and were visualized with alkaline phosphatase-conjugated anti-DIG antibody (Merck) using 4-nitroblue tetrazolium chloride (NBT; Merck) and 5-bromo-4-chloro-3-indolyl phosphate (BCIP; Merck). The sections were observed under a BZ-X800 microscope (KEYENCE, Osaka, Japan).
Immunohistochemistry and hematoxylin and eosin (HE)-staining
View detailed protocolEmbryos at E10.5, E13.5, and E18.5 were fixed and sliced as described above. Depending on the antibody, the sections were antigen retrieved by an ImmunoSaver (Nisshin EM, Tokyo, Japan) for 60 min at 80°C. The sections were incubated with 10% (v/v) fetal bovine serum and 0.4% (v/v) Triton X-100 in HEPES buffer (blocking buffer). After washing, the sections were incubated with primary antibodies (Key resources table) in blocking buffer at 4°C overnight. After the immunoreaction, the sections were incubated with secondary antibodies using Cy3-, Cy5-, or FITC-conjugated AffiniPure donkey anti-goat, rabbit, and mouse IgG (Jackson ImmunoResearch, West Grove, PA). The sections were washed and incubated in VECTASHIELD Mounting Medium (Vector Laboratories, Burlingame, CA) containing 4,6′-diamidino-2-phenylindole dihydrochloride (DAPI). For HE-staining, the sections were stained using standard procedures. The sections were observed under a BZ-X800 fluorescence microscope (KEYENCE).
Scanning electron microscopy (SEM)
Request a detailed protocolWild-type and Dyrk2-/- embryos at E10.5 were washed with 0.1 M phosphate buffer (PB) (pH7.5) and fixed with 2% glutaraldehyde (TAAB Laboratories Equipment, Berkshire, England) in 0.1 M PB (pH 7.4) for 1 week at 4°C. The embryos were placed in tannic acid in 0.1 M PB for 2 hr at room temperature in darkness, and then immersed in 1% OsO4 solution for 2 hr at room temperature. After dehydration in graded ethanol, the samples were transferred into isoamyl acetate and dried at the critical point in liquid CO2, and this was followed by a metal coating procedure (Hitachi, Tokyo, Japan). The surfaces of tissues were then observed using scanning electron microscopy (Hitachi).
Plasmid constructs
Request a detailed protocolFull-length cDNA fragments of mouse Dyrk2 and Aurka were amplified by PCR and cloned in frame into the pFN22K-HaloTag-CMVd1-Flexi-vector (Promega, Madison, WI) and pEGFP-C1 (TaKaRa Bio, Otsu, Japan), respectively. The nucleotide sequences of the primers used are listed in Table 2.
Cell culture and transfection
Request a detailed protocolPrimary mouse embryonic fibroblast (MEFs) were generated from wild-type and Dyrk2-/- embryos at E13.5. MEFs and immortalized human retinal pigment epithelia cells (hTERT-RPE1; Cat# CRL-4000, RRID:CVCL_4388, ATCC, Manassas, VA) were cultured in DMEM (nacalai tesque, Kyoto, Japan) with 10% FBS (biowest, Nuaille, France), 1% GultaMAX (Gibco, Gaithersburg, MD), and 1% Penicillin-streptomycin (nacalai tesque) at 37°C under 5% CO2. hTERT-RPE1 cells were authenticated by the STR profiling and negative for mycoplasma contamination. To induce ciliogenesis, cells were grown to 80–90% confluency and serum-starved (0.5% FBS) for 24 hr. For SAG-stimulation, cells were treated with 100 nM SAG (Merck) for 24 hr after serum-starvation. For rapamycin-stimulation, cells were treated with 0.5 µM rapamycin (LC Laboratories, Woburn, MA) for 24 hr after serum-starvation. Transient knockdown was achieved using the Lipofectamine RNAiMAX transfection regent (ThermoFisher Scientific, Waltham, MA) for 48 hr under serum-starvation conditions according to the manufacturer’s instructions with a final concentration of 6–20 nM siRNA (Key resources table). For over-expression of DYRK2-HaloTag, transfection was performed using X-tremeGENE9 (Merck) for hTERT-RPE1 cells according to the manufacturer’s instructions and the cells were cultured for 24 hr under serum-starvation condition for ciliogenesis. For over-expression of AURKA-EGFP or EGFP, transfection was performed using Xfect (TaKaRa Bio) for MEFs according to the manufacturer’s instructions, and the cells were cultured for 24 hr under serum-starvation condition for ciliogenesis.
Adenovirus infection
Request a detailed protocolAdenovirus construction and infections were performed according to a previous report (Maekawa et al., 2013; Yokoyama-Mashima et al., 2019). Briefly, Flag-DYRK2 and Flag-DYRK2-K251R (Taira et al., 2010; Mimoto et al., 2013) were expressed depending upon Cre-expression. Following infection at a MOI (multiplicity of infection) of 100, MEFs were extracted for gene-expression analysis at 60 hr post-infection. MOI for MEFs was determined using an adenovirus construct for GFP-expression.
Immunoblotting
Request a detailed protocolTissues (the limb buds at E13.5) and MEFs were washed in twice and lysed using RIPA buffer containing several inhibitors (1 mM PMSF, 10 µg/ml Aprotinin, 1 µg/ml Leupeptin, 1 µg/ml Pepstatin A, 1 mM Na3VO4, 10 mM NaF, and 1 mM DTT). Equal amounts of protein (5 µg) were resolved on 4–15% Mini-PROTEA TGX Precast Protein Gels (BioRad, Hercules, CA). After electrophoresis, proteins were transferred to PVDF membranes (Merck). Membranes were blocked with 5% skim milk in tris-buffered saline (TBS) containing 0.05% Tween 20 (TBST) or 0.1% casein/gelatin in TBST, depending on the antibody. Primary and secondary antibodies were reacted in each blocking buffer (Key resources table). Signals were detected using a chemiluminescent regent, ImmunoStar LD (Wako). Signals were observed and band intensity was measured using a Fusion-Solo system (M and S Instruments, Tokyo, Japan).
Quantitative real-time polymerase chain reaction (qPCR)
Request a detailed protocolTotal RNAs were prepared from tissues (the limbs of E13.5, the mandibular arches of E10.5, and whole embryos at E9.5) and MEFs using the RNeasy mini kit (QIAGEN, Germantown, MD) or ISOGEN II (Nippon Gene, Tokyo, Japan), respectively. Reverse transcripts were obtained using PrimeScript Reverse Transcriptase (TaKaRa Bio) and subjected to qPCR using a PIKOREAL96 system (ThermoFisher Scientific). Reactions were performed in KAPA SYBR FAST qPCR Master Mix (NIPPON Genetics, Tokyo, Japan) that included 0.2 μM of a specific primer set for each gene (Table 2). Data were calculated by the comparative CT method (ΔCT method) to estimate the mRNA copy number relative to that of Hprt as an internal standard. The DNA sequence of the PCR product was confirmed by nucleotide sequencing (data not shown).
Immunocytochemistry
Request a detailed protocolFor immunocytochemistry, MEFs and hTERT-RPE1 cells were cultured on 8-well chamber slides (ThermoFisher Scientific) coated with Poly-D-lysin (Sigma-Aldrich). Cells were fixed and antigen retrieved depending on the antibody. The primary antibody reaction was performed at an appropriate dilution (Key resources table) in the presence of blocking buffer at 4°C overnight. After immunoreactions, cells were incubated with secondary antibodies using Cy3-, Cy5-, or FITC-conjugated AffiniPure donkey anti-goat, rabbit, and mouse IgG, and chicken IgY (Jackson ImmunoResearch). The cells were then washed and incubated with DAPI. Immunofluorescence was observed under a BZ-X800 fluorescence microscope (KEYENCE).
RNA-Seq
Request a detailed protocolTotal RNAs were prepared from MEFs cultured in the absence or presence of 100 nM SAG for 24 hr using RNeasy mini kit (QIAGEN) with DNase I treatment (QIAGEN). Materials were enriched for polyA sequences, and quantitative RNA-sequencing was performed using an Illumina HiSeq (Illumina, San Diego, CA). Cutadapt v1.9.1 was used to trim and filter reads, and clean data were aligned to the reference genome (ENSEMBLE, GRCm38.97) using the software HISAT 2 (v2.0.1). Relative gene expression was quantified and normalized in a FPKM (fragments per kilobase of transcript per million mapped reads) format.
STRING and gene ontology (GO) analysis
Request a detailed protocolTo determine the presence of interactions/partnerships among downregulated genes in Dyrk2-/- MEFs, protein-protein interaction networks were extracted from the STRING database (https://string-db.org) and drawn by STRING v11. Gene ontology (GO) analysis was also performed using STRING v11 to demonstrate the biological processes enriched in the altered genes. The resulting GO terms that possessed a false discovery rate (FDR) of less than 0.005 were considered as enriched biological processes.
Statistical analysis
Request a detailed protocolEach experiment was confirmed by at least three independent biological replicates per condition. Data are presented as the means ± SEM. Prism seven software (GraphPad, San Diego, CA, USA) was used for statistical analyses. Means between two groups were compared using the Student’s t-test. Multiple inter-group differences were analyzed by one-way ANOVA (analysis of variance) followed by Tukey’s multiple comparison test.
Data availability
Data except for RNA-seq in this study are included in the manuscript and supporting files. Source data files have been provided: Figure 2-source data 1 Figure 2-figure supplement 1-source data 1 Figure 3-source data 1 Figure 3-source data 2 Figure 3-figure supplement 1-source data 1 Figure 3-figure supplement 2-source data 1 Figure 4-source data 1 Figure 4-figure supplement 1-source data 1 Figure 4-figure supplement 2-source data 1 Figure 4-figure supplement 3-source data 1 Figure 6-source data 1 Figure 6-figure supplement 3-source data 1 Figure 7-source data 1 Figure 8-source data 1 Figure 9-source data 1. RNA-seq data have been deposited in Dryad under accession code URL https://doi.org/10.5061/dryad.pnvx0k6j8.
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Dryad Digital RepositoryThe novel ciliogenesis regulator DYRK2 governs Hedgehog signaling during mouse embryogenesis.https://doi.org/10.5061/dryad.pnvx0k6j8
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Article and author information
Author details
Funding
Japan Society for the Promotion of Science (19K16781)
- Saishu Yoshida
Japan Society for the Promotion of Science (17H03584)
- Kiyotsugu Yoshida
Japan Society for the Promotion of Science (18K19484)
- Kiyotsugu Yoshida
Japan Society for the Promotion of Science (16H06276 (AdAMS))
- Kiyotsugu Yoshida
Takeda Science Foundation
- Saishu Yoshida
the Jikei University Research Fund
- Saishu Yoshida
Japan Society for the Promotion of Science (20H03519)
- Kiyotsugu Yoshida
The funders had no role in study design, data collection and interpretation, or the decision to submit the work for publication.
Acknowledgements
We thank Dr. Yuki Kobayashi at Hiroshima University for constructive suggestions. This work was partially supported by JSPS KAKENHI (grant numbers 19K16781 to Saishu Yoshida and 17H03584, 18K19484, and 20H03519 to Kiyotsugu Yoshida), the Platform of Advanced Animal Model Support from MEXT of Japan (to Kiyotsugu Yoshida), the Jikei University Research Fund (to Saishu Yoshida), and the Takeda Science Foundation (to Saishu Yoshida).
Ethics
Animal experimentation: The animal experiment protocol was approved by the Institutional Animal Care and Use Committee of Jikei University (No. 2017-065 and 2018-031), and the studies were performed in accordance with the Guidelines for the Proper Conduct of Animal Experiments of the Science Council of Japan.
Copyright
© 2020, Yoshida et al.
This article is distributed under the terms of the Creative Commons Attribution License, which permits unrestricted use and redistribution provided that the original author and source are credited.
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