Dishevelled (DVL) is the key component of the Wnt signaling pathway. Currently, DVL conformational dynamics under native conditions is unknown. To overcome this limitation, we develop the Fluorescein Arsenical Hairpin Binder- (FlAsH-) based FRET in vivo approach to study DVL conformation in living cells. Using this single-cell FRET approach, we demonstrate that (i) Wnt ligands induce open DVL conformation, (ii) DVL variants that are predominantly open, show more even subcellular localization and more efficient membrane recruitment by Frizzled (FZD) and (iii) Casein kinase 1 ɛ (CK1ɛ) has a key regulatory function in DVL conformational dynamics. In silico modeling and in vitro biophysical methods explain how CK1ɛ-specific phosphorylation events control DVL conformations via modulation of the PDZ domain and its interaction with DVL C-terminus. In summary, our study describes an experimental tool for DVL conformational sampling in living cells and elucidates the essential regulatory role of CK1ɛ in DVL conformational dynamics.
Wnt signaling pathway is one of the signaling pathways, whose dysfunction or deregulation is linked to developmental defects, inherited diseases, and many types of cancer1. Wnt proteins have been shown to activate several Wnt signaling pathways. The best known Wnt/β-catenin (canonical) pathway typically controls cell proliferation and differentiation by the regulation of transcription, whereas other (i.e. non-canonical) branches typically regulate cell polarity and migration by the reorganization of cytoskeleton2,3,4. Wnt signals are transduced via the membrane receptor Frizzled (FZD) and the intracellular protein Dishevelled (Dsh in Drosophila, DVL1–3 in humans). There is a general agreement based on strong genetic evidence in Drosophila3 and mouse5,6 that DVL protein(s) plays a crucial role in all major branches of Wnt signaling and serves as a signaling hub.
All DVL proteins have a conserved architecture consisting of three well-defined domains: an N-terminal DIX domain (Dishevelled and Axin), a central PDZ domain (Post-synaptic Density Protein-95, Disc Large Tumor Suppressor, and Zonula Occludens-1), and a C-terminal DEP domain (Dishevelled, Egl-10, and Pleckstrin). Crystal structures of all three isolated DVL domains are known7,8,9. The regions linking the three domains and the long C-terminus (200 aa) are intrinsically disordered2.
DVL molecules can multimerize to form high-order structures called DVL signalosomes, which are crucial for the subsequent downstream activation of Wnt/β-catenin signaling10,11,12. Signalosome formation is mediated via head-to-tail multimerization of DVL’s DIX domains10 (and/or DIX domain of Axin protein11,12,13). Recently, dimerization via the DEP domain has also been reported and it was proposed that DEP–DEP interaction mediated by domain swapping cooperates with DIX-dependent DVL signalosome formation14.
Several pieces of information suggest that DVL can also interact intramolecularly. Specifically, it has been shown in vitro that at least two regions located in the C-terminus of DVL— (i) a nuclear export signal and (ii) the terminal 7 aa in the C-terminus of DVL—can interact with the PDZ domain15,16,17. These reports suggested that DVL can exist in a closed and open conformation(s) undergoing multiple structural transitions that control DVL function. However, there is neither an experimental approach to study this phenomenon directly nor clear evidence that DVL exists in multiple conformations in vivo.
In this study we use an experimental system that enables the analysis of DVL conformational sampling in living mammalian cells. We design and characterize several biosensors of DVL3 conformation based on fluorescein arsenical hairpin binder (FlAsH)-based Förster resonance energy transfer (FRET). This single-cell FRET method allows site-selective detection of protein conformation dynamics in living cells and has already helped to decipher various biological problems18,19,20. FlAsH is a small organic compound, which recognizes and binds to CCPGCC tag18. The FlAsH–CCPGCC complex becomes fluorescent and can be used as an energy acceptor in the FRET pair with ECFP (enhanced cyan fluorescent protein). The main advantage of the CCPGCC tag is its size—only 6 aa, which reduces interference with the biological function of the protein of interest18. Using FlAsH FRET DVL3 sensors we describe the conformational dynamics of DVL3 in living cells upon Wnt pathway stimulation and the key function of Casein kinase 1 ɛ (CK1ɛ) in this process.
Design and generation of the FRET-based DVL3 biosensors
FlAsH-based FRET represents a powerful technique that allows monitoring of the protein conformation in biological setups, where large tags can interfere with protein complex formation and function18,19,20. FlAsH molecule forms a fluorescent complex with a 6 aa long sequence (CCPGCC) that can be shut off by addition of BAL (British Anti-Lewisite or 2,3-dimercapto-1-propanol)18. The general scheme of how FlAsH-based FRET works is depicted in Fig. 1a and in Supplementary Fig. 1a. We designed and generated four different DVL3 sensors (FlAsH I–IV), which differ in the position of the CCPGCC tag. Each DVL3 sensor contained the ECFP tag at the N-terminus and one CCPGCC internal tag, located in an intrinsically disordered region (IDR) or at the C-terminus of DVL3. The CCPGCC tags were inserted at the most disordered region of each IDR predicted in silico using PONDR-FIT tool21 as shown in Fig. 1b. Biological and signaling properties of all four DVL3 FlAsH sensors were indistinguishable from wild-type (wt) ECFP-DVL3 in the following assays (performed in HEK293 DVL1-2-3−/− cell line22 in order to avoid interaction with endogenous full-length DVL isoforms): activation of the Wnt/β-catenin pathway monitored by Dual Luciferase TopFlash/Renilla reporter gene assay (Supplementary Fig. 1c); CK1ɛ-dependent DVL electrophoretic mobility shift assay (Supplementary Fig. 1d); and changes of DVL subcellular localization induced by CK1ε (Supplementary Fig. 1e). Data are summarized in Fig. 1c.
The ECFP-DVL3 FlAsH I, II, and III (but not IV) sensors showed robust basal intramolecular FRET measure after BAL addition (Fig. 1d, left panel), which suggests that the ECFP and CCPGCC tags are in physical proximity. Since it has been reported that DVL can undergo intermolecular multimerization via its DIX and DEP domains10,14, intermolecular FRET among different DVL3 molecules can also occur. To assess the intermolecular FRET efficiency, we generated N-terminally HA-tagged DVL3 FlAsH I–IV constructs without the N-terminal ECFP tag. Despite the fact that the ECFP and CCPGCC tags (labeled by FlAsH molecule) showed almost complete co-localization in dots for all four sensors (Supplementary Fig. 1b), the intermolecular FRET efficiency was negligible, except FlAsH III (Fig. 1d, right panel). These results demonstrate that ECFP-DVL3 FlAsH I, II, and III sensors represent a useful tool for the analysis of DVL conformation in living cells that is not affected (FlAsH I, II) or only minimally affected (FlAsH III) by intermolecular FRET due to the DVL–DVL oligomerization.
CK1ɛ changes intramolecular FRET in DVL3 sensors
As a result of Wnt pathway activation, DVL is heavily phosphorylated23,24,25,26. It has been further shown that the major DVL kinase responsible for Wnt-induced phosphorylation of DVL27,28,29 is CK1ɛ. In order to analyze whether and how CK1ε affects DVL3 conformation, we (i) used CK1δ/ε inhibitor PF670462 (refs. 29,30) to pharmacologically inhibit endogenous CK1ε and (ii) promoted DVL3 phosphorylation by overexpression of exogenous CK1ε. Such manipulation of CK1ε activity dramatically affects DVL3 properties such as: (i) CK1ɛ-DVL3-mediated activation of the Wnt/β-catenin pathway monitored by Dual Luciferase TopFlash/Renilla reporter gene assay (Fig. 2a); (ii) phosphorylation status of DVL3 assessed either as a phosphorylation-dependent mobility shift on SDS-PAGE or as an increased signal for pS643-DVL3 phosphorylation-specific antibody—a well-defined29 target site for CK1ε (Fig. 2b), and (iii) changes in the subcellular localization of DVL3 (ref. 31) analyzed by immunofluorescence (Fig. 2c). These properties were analyzed for all four ECFP-DVL3 FlAsH sensors (Supplementary Fig. 2a) and were found indistinguishable from wt FLAG-DVL3 (compare Supplementary Fig. 2a and Fig. 2a–c). This result shows that neither ECFP nor CCPGCC tag addition in any of the four sensors affects the biological response of DVL3 to CK1ε.
To determine how CK1ε influences DVL3 conformation sampling, we analyzed basal FRET in ECFP-DVL3 FlAsH I-IV sensors in: (i) cells treated with the CK1δ/ε inhibitor (PF670462, 10 μM), (ii) control cells possessing active endogenous CK1ε, and (iii) cells overexpressing CK1ε (Fig. 2d, for intermolecular FRET efficiency controls see Supplementary Fig. 2b). Changes in CK1ε levels and activity affected FRET efficiency to a different extent for each sensor. The most prominent differences were detected using the FlAsH III sensor, for which the CK1δ/ε inhibitor consistently increased the FRET efficiency, whereas the CK1ε overexpression decreased it. These experiments implied that CK1ε inhibition results in a more compact (i.e. closed) conformation of DVL3, while CK1ε overexpression leads to a looser (i.e. open) conformation. In order to dissect mechanistically how CK1ε affects the DVL conformations in vivo, we selected DVL3 FlAsH III sensor for a rigorous investigation.
Identification of DVL3 regions in direct contact with CK1ɛ
As a next step, we mapped in detail the interaction site(s) of DVL3 and CK1ε, in order to generate DVL3 variants incapable of CK1ε binding while keeping all structured domains intact. We hypothesized that IDRs significantly contribute to the interaction of DVL3 and CK1ε. The binding epitopes within IDRs are typically defined by linear peptide motifs32 that can be rapidly analyzed in peptide microarrays. For our purposes, we designed a peptide microarray (13-meric peptides overlapping by 10 residues) covering the IDRs of DVL3 (Fig. 3a).
The human DVL3 peptide library also contained phosphorylated versions of those peptides, where phosphorylation sites for CK1ε were previously identified29 (Supplementary Fig. 3). After incubation with recombinant CK1ε, we discovered three peptide clusters—named RGCF (aa 339–351), RGPR (aa 611–623), and FRMA (aa 698–710)—as potential interaction sites with CK1ε (Fig. 3b). The MS/MS-based analysis of the wild-type DVL3 overexpressed in HEK293 cells showed that serine residues in these regions (S350 in RGCF; S611, S612, and S622 in RGPR) were only negligibly phosphorylated, in contrast to S700 in FRMA that was found constitutively phosphorylated (Supplementary Fig. 4b). When CK1ε was overexpressed, all residues in RGCF and RGPR regions were phosphorylated (Supplementary Fig. 4c, d). Importantly, phosphorylated variants of these peptides showed negligible interaction with CK1ε in the peptide array (Supplementary Fig. 4e). The quantification of the in vitro binding between the peptides corresponding to these regions and recombinant CK1ε using fluorescence anisotropy (FA) showed affinities close to 1 µM for all three peptides but negligible interaction for their phosphorylated variants (Supplementary Fig. 4a). This suggests that the interaction is phosphorylation-sensitive and CK1ε is released once the binding epitopes get phosphorylated.
Deletion of these regions in DVL3 (hereafter referred as DVL3 ΔALL variant) (Fig. 3c) drastically reduced, but not completely abolished, the interaction with CK1ε as confirmed by coimmunoprecipitation and resulted in the diminished phosphorylation at the CK1ε target site S643 (Fig. 3d–g). Functionally, DVL3 ΔALL failed to activate the downstream Wnt/β-catenin pathway in the TopFlash reporter assay (Fig. 3h) in HEK293 DVL1-2-3−/− cells.
Intriguingly, the DVL3-CK1ɛ-binding sites show high sequence conservation (Fig. 3b, top) and are almost identical in humans and Xenopus (Fig. 3i). This allowed us to analyze the functional consequences of these deletions also in vivo. The activation of the Wnt/β-catenin pathway results in the axis duplication in Xenopus, which is a well-defined functional Wnt/β-catenin signaling readout (Fig. 3j, left). First, we injected a dose of mRNA encoding Dvl3 wild type into the marginal zone of the ventral blastomeres of the four-cell stage Xenopus laevis embryos to induce double axis formation (Fig. 3j, right). Not surprisingly, the xDvl3 ∆ALL variant (lacking aa 338–350, 609–619, and 693–705 in xDvl3) showed dramatically reduced capacity to induce axis duplication both in the presence and absence of exogenous xCK1ɛ (Fig. 3j, right). Taken together, these data demonstrate that the identified DVL3 regions represent evolutionary conserved bona fide interaction sites for CK1ɛ, whose deletion abolishes both CK1ɛ binding and CK1ɛ-dependent functions of DVL3.
CK1ε is required for the conformational dynamics of DVL3
As the DVL3 ΔALL variant is incapable of complete interactions with CK1ɛ, we further examined the role of CK1ε in the conformational dynamics of DVL3. Using the FlAsH III sensor as a template, we generated and analyzed the ECFP-DVL3 FlAsH III ∆ALL variant (Fig. 4a). Conformational dynamics of DVL3 ∆ALL was lost but, interestingly, the FRET efficiency for all three conditions was low—suggesting that DVL3 ∆ALL remains in the open rather than the closed conformation. To further analyze this phenomenon, we produced CK1ɛ-deficient (CK1ɛ−/−) HEK293 cells using the CRISPR-Cas9 system (Fig. 4b). These cells (Fig. 4b) failed to respond to Wnt ligands as demonstrated by the lack of phosphorylation of DVL2 and DVL3, and pS1490-LRP6. DVL3 overexpression in CK1ɛ−/− cells failed to induce Wnt/β-catenin pathway activation monitored by TopFlash in the absence of exogenous CK1ɛ (Supplementary Fig. 4f). Importantly, the FRET efficiency of the DVL3 FlAsH III sensor in CK1ɛ−/− cells was low and CK1ɛ inhibition was unable to increase it as it did in HEK293 wt cells (Fig. 4c). These data suggest that DVL3 in the absence of CK1ε remains in an open (and non-phosphorylated) rather than a closed (and non-phosphorylated) conformation that is observed when CK1ε is present but inhibited by the CK1δ/ε inhibitor PF670462. One explanation can be non-specific effects of CK1δ/ε inhibitor PF670462, unrelated to CK1ε inhibition. To exclude this possibility, we overexpressed dominant negative (dn) CK1ε mutant P3, which efficiently binds to DVL3 (ref. 33). The presence of dnCK1ε as well as wild-type CK1ε in combination with PF670462 inhibitor resulted in the significantly increased FRET signal of the DVL3 FlAsH III sensor (Fig. 4d). This confirmed that in presence of inactive CK1ε, DVL3 adopts a more compact conformation which is not the case when CK1ε is absent from the DVL3 complex. In summary with other results, it suggests that CK1ɛ has a dual role: (i) it retains DVL3 in a compact conformation by physical interaction and (ii) triggers a phosphorylation-induced open conformation of DVL3, when activated.
C-terminus-PDZ interaction controls conformations of DVL3
The recent study by Lee et al.16 has proposed that DVL can switch between open and closed conformations. Using mouse Dvl1 they demonstrated that the closed conformation results from the binding of the conserved terminal 7 aa of the C-terminus (EFFVDIM sequence) to the PDZ domain (for schematics see Fig. 5a). Therefore, we asked whether this interaction contributes at least partially to the DVL3 conformational dynamics detected by our FRET sensor. Indeed, DVL3 lacking the very C-terminal part (the ∆C variant of DVL3 FlAsH III, which lacks aa 699–716; Supplementary Fig. 5b) showed significantly lower basal FRET efficiency than wt DVL3 FlAsH III (Fig. 5b). This suggests that the interaction between the C-terminus and PDZ may play a role in the conformational sampling of DVL.
Our next question was whether CK1-mediated phosphorylation in the PDZ domain and the C-terminus contributes to the conformational dynamics induced by CK1ε. First, we employed the MS/MS approach to analyze the phosphorylation of DVL3 induced by CK1ε in the PDZ domain of DVL3. Two phosphorylation sites highly induced by CK1ε were found in the PDZ domain: S268 and S311 in DVL3 immunoprecipitated from HEK293 cells (Fig. 5c) as well as in the in vitro purified full-length DVL3 phosphorylated by recombinant CK1ε in vitro (Fig. 5d). Furthermore, C-terminal S700 in DVL3 was found to be constitutively phosphorylated in HEK293 cells, as previously mentioned (Supplementary Fig. 4b). All three serine residues are fully conserved (Supplementary Fig. 5a, b). To investigate how the phosphorylation status of S268 and S311 in the PDZ domain influences DVL3 conformation, we created ECFP-DVL3 FlAsH III wt construct that was either non-phosphorylatable (S268A/S311A) or phosphorylation-mimicking (S268E/S311E). DVL3 FlAsH III S268A/S311A variant showed higher FRET efficiency indicating the closed conformation, whilst the FRET efficiency of the DVL3 FlAsH III S268E/S311E variant was lower (Fig. 5e), suggesting predominantly the open conformation for this variant. Intriguingly, the FRET efficiency was not significantly affected by the CK1ε inhibition or CK1ε overexpression in any of these variants (Fig. 5e).
Altogether, these data suggest that the CK1-induced phosphorylation of S268 and S311 can control the conformation of DVL3. This led us to investigate whether this regulation can be explained at the atomic level as a result of weaker binding of the (phosphorylated) C-terminus to the PDZ domain phosphorylated at S268 and/or S311.
PDZ domain phosphorylation regulates the C-terminus binding
We performed in silico simulations to investigate the interaction between the C-terminal peptide of human DVL3 (aa 709–716) and human DVL3 PDZ (aa 245–338) domain. We found that the C-terminal peptide binds to the PDZ domain in the canonical binding groove (primary binding site34) forming an antiparallel β-strand with β2-strand of the PDZ domain (Fig. 6a). Moreover, this interaction extends to the β2–β3 loop, where S268 via its hydroxyl forms a hydrogen bond with the carboxyl group of E710 (Fig. 6b). β2–β3 Loop has been reported as an additional binding site in the PDZ domains of several other proteins34,35,36 but in DVL, such interaction (S268-E710) has not yet been reported.
To estimate the effect of phosphorylation on peptide binding in silico, we investigated the interaction between the peptide and the DVL3 PDZ with two phosphorylated serines (pS268/pS311), phosphomimic S268E/S311E, and non-phosphorylatable S268A/S311A. In all cases, the peptide remained bound to the PDZ during the entire simulation (500 ns). However, the enthalpic interaction between the PDZ and the peptide were weaker for both phosphorylated and the mimetic variant by roughly 20% when compared to PDZ wt (Fig. 6c, d). In contrast, the alanine double mutant showed similar interaction strength as wt (Fig. 6e). The changes to the interaction strength were mostly situated in proximity to mutated/phosphorylated sites in the β2–β3 loop with a minor change in the primary carboxyl binding site (see Fig. 6b). The observed interaction strengths correlate with the preference of each PDZ mutant for open or closed conformation observed in the in vivo experiments and provide a candidate mechanism supporting FRET experimental observations.
In order to address the possible role of DVL3 phosphorylation-driven regulation involving S268 and S311 in vitro, we performed NMR structural characterization (Fig. 6f–i). For this purpose, we exploited the well-characterized PDZ domain of human DVL2 (aa 265–361)14, where S286 and S329 correspond to S268 and S311 of human DVL3. Investigation of chemical shift differences revealed that the phosphorylation-mimicking substitutions (S286E/S329E) do not affect the PDZ fold16 (Supplementary Fig. 6a–c). Next, we performed NMR titrations with a phosphorylated (pS700) C-terminal peptide ligand derived from DVL3 (aa 698–716). The phosphorylation variant was chosen as the most physiological, since S700 appeared as constitutively phosphorylated (see Supplementary Fig. 4b). The peak trajectories induced by peptide binding are linear and follow the same course for both PDZ wt and phosphorylation-mimicking variant indicating a similar binding mode. Of the two serine residues, only S286 is affected by peptide binding and clearly experiences larger perturbation than its glutamic acid counterpart (Fig. 6f, Supplementary Fig. 6d). This is in line with in silico data, proposing that S286 in DVL2 (corresponding to S268 in DVL3) is directly involved in contacts with the C-terminal peptide.
Intermediate and intermediate-to-fast exchange peaks correspond to PDZ residues of the binding groove (Fig. 6g). These residues experience severe line broadening throughout the course of the ligand titration in PDZ wt when compared to S286E/S329E variant (Fig. 6i). Fast exchange peaks correspond to residues at the groove periphery. Their quantitative analysis shows that the phosphorylation-mimicking variant has a two-fold weaker affinity for the peptide (Fig. 6h). In principle, the chemical shift perturbations are larger for PDZ wt, indicating that the equilibrium is shifted further to the bound state when compared to the PDZ phosphorylation-mimicking variant (Supplementary Fig. 6d). As an independent confirmation of this conclusion, we also performed surface plasmon resonance (SPR) binding experiments (Fig. 6j). The apparent dissociation constants derived from SPR are in line with the NMR observations and reported a two-fold lower peptide affinity for the PDZ phosphorylation-mimicking variant.
In summary, the biophysical data and the in silico simulations indicate a phosphorylation-driven mechanism that modulates the binding of DVL C-terminus to PDZ domain. In combination with other results in this study, we propose that such mechanism contributes to the CK1-dependent control of DVL conformational changes.
Wnt ligands promote open conformation of DVL3
It has been shown previously that stimulation with Wnt ligands activates CK1δ/ε that in turn phosphorylate DVL. Wnts from both major groups—i.e. capable to activate Wnt/β-catenin (i.e. Wnt-3a) or alternative non-canonical Wnt pathway (i.e. Wnt-5a)—trigger phosphorylation of DVL that is dependent on CK1δ/ε activity (Fig. 7a). Thus, we decided to test if/how Wnts change the conformation of DVL3. To do this, we generated two stable cell lines (derived from HEK293 wt and HEK293 DVL1/2/3 triple knockout22 cells) utilizing tetracycline-controlled promoter driving expression of ECFP-DVL3 FlAsH III sensor (Fig. 7b, c). Under these conditions, the ECFP-DVL3 FlAsH III gets expressed at levels comparable to endogenous DVL3 (Fig. 7c), and in response to Wnt stimulation gets phosphorylated—this can be monitored either as a phosphorylation-dependent shift or by anti-phospho-S643 antibody (Fig. 7d). Analysis of FRET efficiency in both cell lines showed that basal FRET efficiency (≈2%) was comparable with the control conditions analyzed upon transient overexpression of ECFP-DVL3 FlAsH III (see Figs. 2 and 4). Importantly, treatment with both Wnt-3a and Wnt-5a resulted in significantly lower FRET, regardless of the cell line used (Fig. 7e, f). Altogether, these results show that stimulation with Wnt ligands changes DVL3 conformation similarly to the overexpression of CK1ε and suggest that the phosphorylation-driven conformational switch participates in the mechanism of Wnt-induced DVL activation.
Open DVL3 is evenly localized and better membrane recruited
Our analyses of DVL3 conformational dynamics by FRET identified multiple conditions that promote either open or closed conformations of DVL3 (see Figs 2, 4 and 5). These conditions/mutations (schematized in Fig. 8a) include changes in the CK1ε activity, presence/absence of DVL3 C-terminus, phosphomimicking/blocking mutations in the PDZ domain, capacity of DVL3 to interact with CK1ε, and presence or absence of CK1ε in cells. Altogether, we could identify five cases associated with open conformation and three cases associated with closed conformation. In order to link DVL3 conformational changes with its biological properties, we decided to perform a systematic correlative analysis. The following conditions were included as closed: DVL3 wt + CK1δ/ε inhibitor PF-670642, DVL3 wt + dnCK1ε, and DVL3 (S268A/S311A), or open: DVL3 wt + CK1ε wt, DVL3 ΔALL, DVL3 (S268E/S311E), DVL3 ΔC, and DVL3 wt in CK1ε−/− cells.
First, we analyzed the preferred subcellular localization of DVL3 (as introduced in Fig. 2c)10,14. As shown in Fig. 8b, the open variants of DVL3 are significantly more evenly distributed whereas closed DVL3 is more punctate. Next, we investigated if DVL3 conformation correlates with the capacity of DVL3 to be recruited by FZD6, a key Wnt receptor, to the plasma membrane. For this purpose, we co-expressed FZD6 and analyzed membrane recruitment of DVL3 in FZD6-positive cells by immunofluorescence37. Individual cells were categorized as: not recruited (Fig. 8b, no DVL3 in the membrane), partially recruited (clear membrane as well as cytoplasmic localization), and fully recruited (predominantly plasma membrane localization, Fig. 8c, left). This analysis showed that closed DVL3 is less efficiently recruited to the membrane by FZD6, whereas open DVL3 behaves either as a control or is recruited more efficiently (Fig. 8c). In the last readout we analyzed the capacity of DVL3 to activate downstream Wnt/β-catenin pathway monitored by TopFlash reporter assay (Fig. 8d). Under all conditions where DVL3 is closed—DVL3 (S268A/S311A), DVL3 wt + CK1δ/ε inhibitor, and DVL3 wt + dnCK1ε—no (or negligible) TopFlash/Renilla activation was observed. On the other hand, under conditions that favor the open conformation both activation as well as inhibition of the Wnt/β-catenin pathway was evident.
Next, we plotted the biological properties of individual open and closed cases in a single graph (Fig. 8e, f; Supplementary Fig. 7a). When both subcellular localization and FZD6-induced membrane recruitment were considered, open and closed conditions separated from wt DVL3 very clearly (Fig. 8e). Ability to activate TopFlash was observed only when CK1ε was co-expressed with wt DVL3. Thus, it seems that CK1ε activity represents an independent additional factor that controls the behavior of open DVL3 forms; i.e., open conformation is not sufficient (although it can be required) for DVL3 to activate downstream Wnt/β-catenin signaling. Altogether these data demonstrate a strong correlation between DVL3 conformations and their ability to be recruited to the receptor complex (FZD6) or localize evenly in a cell.
In the cell culture model we were unable to dissect the effects on the non-canonical Wnt/PCP pathway, and as such we turned into the Xenopus embryo model. Alterations in the Wnt/PCP pathway activity result in the convergent extension (CE) defects (Supplementary Fig. 7b, right). In order to avoid any artifacts, we tested the constitutively open and closed variants of xDvl3 based on point mutations or small deletions—namely open xDvl3 ΔC and xDvl3 (S267E/S310E) and closedxDvl3 (S267A/S310A). Phosphorylation sites in the PDZ domain are fully conserved between human and Xenopus (for alignment see Supplementary Fig. 5a) and hDVL3 S268/S311 corresponds to xDvl3 S267/S310. As shown in Supplementary Fig. 7b, open variants of xDvl3 showed similar potency to induce CE defects as wt xDvl3 with approximately 70–80% embryos displaying CE phenotype, whereas the closed xDvl3 (S267A/S310A) showed significantly reduced capacity to induce CE/NT (neural tube) defects with less than 50% affected embryos. These results correlate strongly with the capacity of the corresponding human DVL3 variants to be recruited to the membrane by FZD6 (Fig. 8c).
In this study we establish an FlAsH-based single-cell FRET tool for the investigation of DVL conformations in intact living cells. Using this approach, we identify a key role of CK1ε, a major DVL kinase, in controlling DVL conformation in vivo.
The concept of DVL conformational sampling was first introduced by Jung et al.38. They proposed that the C-terminus of DVL is a ubiquitin-binding domain that can recognize K63-linked ubiquitin chains in the DEP domain to yield an inactive, closed, conformation38. Subsequent studies of Zheng group16,17, in vitro proposed an alternative open/closed conformational switch mediated by docking of the C-terminus to the PDZ domain of DVL. The FlAsH-based FRET DVL3 sensor technique allows us to identify a key role of phosphorylation in the regulation of this process. Specifically, we identify two CK1ε-induced phosphoserine residues (S268 and S311 in human DVL3) in the PDZ domain whose mutation dramatically interferes with the DVL3 conformational sampling, and further supports the C-terminus–PDZ interaction model16,17.
Previously, we have shown28 that efficient interaction of DVL3 and CK1ɛ requires multiple DVL3 regions. The DIX domain is the only region of DVL3 which seems to be dispensable for high affinity interaction28. The DEP domain appears to be the most important structured domain involved in CK1ɛ binding28,39; here we identify three regions in the IDRs of DVL3 that are involved in CK1ɛ interactions. DVL3 lacking these three short sequences is not only inefficient to bind CK1ε but it is also not amenable to conformational rearrangements. Interestingly, such DVL3 variant is found counterintuitively in the open conformation. The same applies when CK1ε is eliminated in the CK1ɛ−/− cell line. This suggests that CK1ɛ can also have an important scaffolding function required to retain DVL3 in the closed conformation. This view is schematized in Fig. 9. Similar function has been observed for other kinases that regulate biological processes not only by their catalytic activity but also by their scaffolding function40. In principle, the requirement for CK1 as a scaffold can help to elucidate earlier findings shown by genetic experiments in Drosophila that Wnt/PCP pathway requires CK1ɛ but not its kinase activity (in contrast to Wnt/β-catenin pathway that requires both)41.
The key question is how DVL conformation affects the formation of Wnt signaling complexes. We can show that both Wnt-3a, which triggers Wnt/β-catenin pathway, and Wnt-5a ligand, which activates non-canonical Wnt pathway, promote open conformation of DVL3. Both these ligands activate CK1ε, which results in a very similar or identical phosphorylation of DVL24. At the same time, we could correlate open conformations of DVL3 with the efficient FZD6-dependent membrane recruitment of DVL3. A similar correlation was reported recently using XDsh, XFz7, and zebrafish embryonal cells17. Based on these facts, we propose a model where Wnt-induced activation of CK1ε leads to the phosphorylation of S268/S311 in the PDZ domain and an open DVL conformation; i.e. open DVL3 then gets more efficiently bound to FZD. The molecular mechanism behind the more efficient recruitment to FZD-centered receptor complex is unknown but several candidate mechanisms reported in the literature can be considered for further testing. First, it is possible that in a closed conformation (i.e. when the binding groove of PDZ is occupied by DVL C-terminus), a conserved KTXXXW motif in the C-termini of FZDs that is capable of direct interaction with the PDZ42,43 domain cannot interact with DVL. Second, the liberation of the DVL C-terminus in the open conformation provides a binding interface that can be recognized by proteins that facilitate receptor complex assembly. Such a candidate In the non-canonical Wnt pathway could be Ror2, which binds the C-terminus of DVL and more efficiently recognizes DVL phosphorylated by CK1 (ref. 44). Third, our data show that the closed variants of DVL3 are more punctate whereas open variants are more evenly distributed. These phenotypes approximate the multimerization properties of DVL mediated by DIX and DEP domains10,14. In all our conditions, DVL3 has intact DIX and DEP domains, which suggests that the conformation itself affects multimerization and/or biophysical properties of DVL. One can speculate that closed DVL3 represents an inactive and immobile pool of DVL whereas open DVL is more mobile. Existing reservoirs of inactive or autoinhibited DVL have been proposed before17,45—for example: DVL-binding protein nucleoredoxin (NXN) can recognize such a pool and prevent it from degradation45,46. The key function of CK1 upon activation of Wnt pathway can then be mobilization of DVL from the inactive pool to be followed by FZD-mediated events—this distinction is in line with earlier findings showing that the action of CK1ε and FZD on DVL is molecularly distinct29.
Taken together, we provide evidence that Wnts and CK1ε regulate the conformation of DVL3, and that DVL3 in the open conformation, induced by these stimuli, is more mobile and more efficiently recruited to FZD. The FlAsH FRET DVL3 sensor technique provides the tool for the follow-up studies that can shed light on the diverse DVL functions at the membrane, in the centrosome, in the nucleus, and mainly on the regulation of DVL function in the Wnt/β-catenin and Wnt/PCP signaling pathways.
Cell culture and transfection and mutagenesis and treatments
HEK293 wild type (ATCC-CRL-11268), DVL1-2-3−/− (published in ref. 22), ECFP-DVL3 FIII and CK1ɛ−/− cell lines (both derived from the aforementioned HEK293 wild-type cells) were grown at 37 °C and 5% (vol/vol) CO2 in Dulbecco’s modified Eagle’s medium (DMEM; Gibco #41966-029), 10% (vol/vol) fetal bovine serum (Gibco, #10270), 2 mM l-glutamine (Life Technologies, #25030024), and 1% (vol/vol) antibiotics (penicillin/streptomycin; Hyclone-Biotech, #SV30010).
For immunofluorescence, cells were seeded (40,000 per well) on 24-well plates with gelatin-coated coverslips and transfected, as indicated, with 0.1 μg of each corresponding plasmid (0.3 μg of mCherry-FZD6) for 6 h. For western blotting and Dual Luciferase TopFlash/Renilla Reporter Assay, cells were seeded (60,000 per well) directly on 24-well plates with 0.1 μg of each corresponding plasmid (if not indicated otherwise) for 6 h. For coimmunoprecipitation, cells were seeded (4.4 × 106) on 10-cm dishes and transfected with 1 μg of each corresponding plasmid. The next day after seeding, cells were transfected using polyethyleneimine (PEI) in a stoichiometry of 6 μl of PEI per 1 μg of DNA for 6 h and were harvested 24 h after transfection. The following plasmids used in HEK293 cells have been described previously: FLAG-DVL3 wt47, CK1ϵ wt48, mCherry-FZD6 (ref. 37), and dominant-negative CK1ϵ P3 (ref. 33). The ECFP-DVL3 wt plasmid was made by Gateway Technology (via LR recombination according to the manufacturer’s instructions; Thermo Fisher Scientific, #11791020) from the donor plasmid pDONR221 DVL3 (DNASU, #FLH178665.01x) and the destination plasmid pdECFP (LMBP, #4548). The HA-DVL3 wt plasmid was made by Gateway Technology from the donor plasmid pDONR221 DVL3 (DNASU, #FLH178665.01x) and the destination plasmid pcDNA3.1 N-term HA (gift from Erich Nigg).
Mutagenesis reactions were performed using the QuikChange II XL Site-Directed Mutagenesis Kit following the manufacturer’s instructions (Agilent Technologies, #200521). All mutations described in this study were verified by Sanger sequencing. All primers used for the site-directed mutagenesis are listed in Supplementary Table 1. All plasmids and more detailed information are available upon request.
Cells were treated as indicated by 10 μM CK1δ/ϵ inhibitor PF-670642 (Santa Cruz, #sc-204180A) overnight; 1 μM LGK974 Porcupine inhibitor (Stem RD, #974-02) overnight; 1 µg/ml of tetracycline for 4 h; and by Conditional Media (CM) for 3 h (WB, FlAsH-based FRET approach) or 8 h (TopFlash/Renilla Dual luciferase assay), which were obtained from the control or Wnt-3a/Wnt-5a stably overexpressing L-cells mouse cell line (L-Wnt3a; ATCC-CRL-2647 and L426 Wnt5a cells; ATCC-CRL-2814) according to the ATCC instructions.
CRISPR-Cas9 generation of HEK T-REx-293 CK1ε−/− cell line
The sequence of gRNA targeting CSNK1E gene was chosen according to Broad Institute CRISPRko designing tool as follows: gRNA (CSNK1E)—AAGTTCTACAAGATGATGCA(GGG) (SfaNI restriction site indicated, PAM sequence in brackets).
The following plasmids were used for gRNA cloning: pSpCas9(BB)-2A-GFP (PX458) (Cas9 from S. pyogenes with linked EGFP and cloning backbone for gRNA, Addgene plasmid #48138)49 and pU6-(BbsI)_CBh-Cas9-T2A-mCherry (Cas9 from S. pyogenes with linked mCherry and cloning backbone for gRNA, Addgene plasmid #64324)50.
T-REx-293 cells (Invitrogen) were cultured according to the manufacturer’s instructions and transfected by Lipofectamine® 2000 DNA Transfection Reagent (Thermo Fisher Scientific) with #48138 (cloned in gRNA for CSNK1E). Cells were subsequently subjected to FACS (fluorescence activated cell sorting) where simultaneously GFP (green fluorescent protein) and mCherry-positive cells were seeded in 96-well plates in one cell per well format.
Monoclonal cell lines were backed up and subsequently screened by western blot using CK1ε antibody (Santa Cruz, #sc-6471). For verification and specification of modification were above-mentioned PCR products cloned into pcDNA3 plasmid (Invitrogen) and sequenced using CMV forward primer: CGCAAATGGGCGGTAGGCGTG.
Generation of HEK T-REx-293 ECFP-DVL3 FlAsH III cell lines
cDNA encoding ECFP-DVL3 FlAsH III was amplified by Pfx50 DNA Polymerase (Thermo Fisher Scientific, #12355012) using primers containing sequences recognized by HindIII (forward primer TATAAGCTTatggtgagcaaggg; HindIII site underlined) and XbaI (reversed primer AATTCTAGAtcacatcacatccacaaa; XbaI site underlined) restriction enzymes (Thermo Fisher Scientific, #ER0501 and #ER0681), extracted from gel using GeneJET Gel Extraction Kit (Thermo Fisher Scientific, #K0691) and ligated into HindIII- and XbaI-linearized pcDNA4/TO (Thermo Fisher Scientific, #K102001) vector using T4 DNA Ligase (New England Biolabs, #M0202) according to the manufacturer’s protocol. Then competent E. coli DH5α bacteria were transformed with ligation mix using standard heat-shock protocol, individual bacterial colonies were picked, cultured, and plasmid DNA was isolated by GenElute Plasmid DNA Miniprep Kit (Sigma-Aldrich, #PLN70). Plasmids were checked by Sanger sequencing (forward sequencing primer ATTGACGCAAATGGGCG; reverse GCCTTCCTTGACCCTGGA) for the presence of the ECFP-DVL3 FlAsH III wt cDNA. Next, T-REx-293 cells (Invitrogen) and their derivate HEK293 DVL1-2-3−/− cell line22 were transfected with pcDNA-4-TO-ECFP-DVL3 plasmid using PEI. Twenty-four hour post-transfection culture medium was changed for the new one supplemented with 200 μg/ml for generation of stable cell lines. After selection clonal lines were obtained using the serial dilution method and analyzed by western blot using the GFP/DVL3 antibodies for the inducible transgene expression by treatment with 1 μg/ml of tetracycline.
Dual luciferase TopFlash/Renilla Reporter Assay
Cells were transfected 24 h after seeding with 0.1 μg of Super8X TopFlash construct, 0.1 μg of Renilla luciferase construct, and 0.1 μg of corresponding plasmids per well for 6 h in a 24-well plate. As for the ECFP-DVL3 FIII wt stable cell lines, transfection was followed by 4 h induction of tetracycline (1 µg/ml) and 8 h treatment of CM:DMEM (1:1 ratio). For performing this assay, Promega Dual Luciferase assay kit (Promega, #E1910) was used according to the manufacturer’s instructions. Luminescence was measured by a Hidex Bioscan Plate Chameleon Luminometer. Results are depicted as the ratio of TopFlash and Renilla signal (TopFlash fold induction), which was normalized for each experiment to certain control column (normalized TopFlash fold induction). Data were analyzed by MS Excel 2007 and GraphPad Prism 6 and results were shown as the means ± S.D. (number of experiments indicated ad hoc).
Western blot and sample preparation
Coimmunoprecipitation protocol was used modified from Bryja et al.29 DMEM was removed after 24 h, cells were washed by phosphate-buffered saline (PBS) and 1 ml of cold NP40-based lysis buffer (50 mM Tris buffer, pH 7.4; 300 mM NaCl; 1 mM EDTA; 0.5 % NP40) supplemented with 1× protease inhibitors (Roche Applied Science, #11836145001), 0.1 mM DTT and 1× phosphatase inhibitors (Calbiochem, #524625) was used per one 10-cm dish. The lysate was collected after 15 min of lysis on 4 °C and was cleared by centrifugation at 16.1 r.c.f. for 30 min. Samples with the antibody (1.25 µg of antibody per sample) were incubated on carousel overnight. In the morning, 30 µL of G protein-Sepharose beads (GE Healthcare, #17-0618-05)—previously blocked overnight in NP40-based lysis buffer supplemented with 5% bovine serum albumin (BSA) and in the morning equilibrated in BSA-free complete NP40-based lysis buffer—were then added to samples. After 4 h of incubation on carousel, samples were washed four times, 40 µL of 2× Laemmli buffer were added, and samples were boiled. The antibody used for immunoprecipitation was anti-CK1ɛ (BD Biosciences, #610445).
Blot and sample preparation were performed as previously described51 and developed using chemiluminescence documentation system FusionSL (Vilber-Lourmat). The antibodies used were: anti-FLAG M2 (1:1000; Sigma-Aldrich, #F1804), anti-FLAG (1:1000; Sigma-Aldrich, #F7425), anti-DVL3 (1:1000; Santa Cruz, #sc-8027), anti-DVL3 (1:1000; Cell Signaling, #cs-3218S), anti-DVL2 (1:1000; Cell Signaling, #cs-3216S), anti-CK1ɛ (1:500; BD Biosciences, #610445), anti-CK1ɛ (1:500; Santa Cruz, #sc-6471), anti-GFP (1:2000; Fitzgerald, #20R-GR-011), anti-LRP6 pS1490 (1:250; Cell Signaling, #cs-2568), anti-tubulin (1:2000; Sigma-Aldrich, #T6199), anti-DVL3 phospho S643 (ref. 29) (1:1000), and anti-DVL3 phospho S697 (ref. 52) (1:1000). All relevant uncropped blots are available in the Source Data file.
Cells were seeded on gelatin-coated coverslips in 24-well plates and were transfected the next day. Cells were fixed 24 h later in fresh 4% paraformaldehyde, permeabilized with 0.5% Triton X-100, blocked with PBS/BSA/Triton/Azide buffer (PBTA) [3% (wt/vol) BSA, 0.25% Triton, 0.01% NaN3] for 1 h, and incubated overnight with primary antibodies (in dilution 1:500) in PBTA at 4 °C. The next day, the coverslips were washed in PBS and incubated with secondary antibodies conjugated to Alexa Fluor 488 (Invitrogen A11001) or/and Alexa Fluor 594 (Invitrogen A11058) (all in dilution 1:1000), washed with PBS [in case of samples containing FLAG-DVL3 WT and derived variants stained with DAPI (1:5000)], and all coverslips were mounted on microscopic slides. Cells were then visualized on an Olympus IX51 fluorescent microscope using ×40 air or ×100 oil objectives and/or an Olympus Fluoview 500 confocal laser scanning microscope IX71 using ×100 oil objective. One hundred positive cells per experiment (n = 3) were analyzed and scored according to their phenotype into two/three categories (punctae/even); or non-recruited/partially/fully recruited for FZD6-dependent recruitment of DVL3. The antibodies used were as follows: anti-FLAG M2 (Sigma-Aldrich, #F1804), anti-DVL3 (Santa Cruz, #sc-8027), anti-CK1ɛ (Santa Cruz, #sc-6471), anti-RFP (Chromotek, #5h9) and anti-GFP (Fitzgerald, #20R-GR-011).
Xenopus laevis embryos
The work with Xenopus laevis was carried out according to the German animal use and care law (Das Tierschutzgesetz) and approved by the local authorities and committees (animal care and housing approval: I/39/EE006, Veterinäramt Erlangen; animal experiments approval: 54-2532.2-8/08, German state administration Bavaria/Regierung von Mittelfranken). The generation and cultivation of Xenopus embryos was done in accordance with general protocols and staged after the normal table of Niewkoop and Faber (1994)53.
RNA for microinjection was synthesized from plasmids pCS2 myc-xDvl3 (ref. 54), pCS2 myc-xDvl3 ΔALL (lacking sequence corresponding to aa 338–350, 609–619, and 693–705 in xDvl3), pCS2 xDvl3 (S267A/S310A), pCS2 xDvl3 (S267E/S310E), pCS2 xDvl3 ΔC, and pCS2 xCK1ε55, respectively, using the mMessage mMachine Kit (Ambion). Embryos were injected at the four-cell stage either into the two ventral blastomeres for testing the constructs' ability to induce a secondary body axis. Injection amounts of synthetic RNA were 500 pg for myc-xDvl3 wild type and the myc-xDvl3 ∆ALL variant, and 150 pg for xCK1ε RNA. For the analysis of morphogenetic defects, four-cell stage embryos were injected into the two dorsal blastomeres with 100 pg myc-xDvl3 RNA and the corresponding variant RNAs. After injection, the embryos were cultivated until they reached stage 26, fixed, and analyzed for axis duplication or morphogenetic defects, respectively.
HEK293 cells were seeded onto round 24-mm coverslips, which were previously placed in six-well plates and coated with 200 μl of poly-d-lysine (1 mg/ml) for 20 min. Cells were transfected 16–18 h later using Effectene (Qiagen), according to the manufacturer’s instructions. DMEM was replaced 6 h later and the analysis was done 24 h after transfection. As for the ECFP-DVL3 FIII stable cell lines: next day after seeding, protein expression was induced by 4 h treatment of tetracycline (1 µg/ml), which was followed by 3 h treatment of CM:DMEM (1:1 ratio).
FlAsH labeling of the DVL3 FlAsH sensors was performed as previously described18,19. In summary, transfected cells were washed once with Hank’s Balanced Salt Solution (HBSS) containing 1.8 g/l glucose and then incubated at 37 °C for 1 h with HBSS supplemented with 500 nM FlAsH; 12.5 μM 1,2-ethanedithiol (EDT); and corresponding inhibitors. In order to reduce non-specific labeling, cells were then rinsed once with HBSS and incubated for 10 min with HBSS containing 250 µM EDT and corresponding inhibitors. Last, cells were washed twice with HBSS and maintained in DMEM medium with corresponding inhibitors (for the ECFP stable cells —CM:DMEM (1:1 ratio)).
Fluorescence imaging was performed as previously described18,56. To determine the FRET efficiency of the DVL3 FlAsH sensors, coverslips with the cells were mounted using an Attofluor holder (Molecular Probes) and placed on a Zeiss inverted microscope (Axiovert200), equipped with ×63 oil objective lens and a dual-emission photometric system (Till Photonics). Cells were excited at 436 ± 10 nm using a frequency of 10 Hz with 40 ms illumination time out of a total of 100 ms. Emission of ECFP (480 ± 20 nm) and FlAsH (535 ± 15 nm), and the FRET ratio (FlAsH/ECFP) were monitored simultaneously. Fluorescence signals were detected by photodiodes and digitalized using an analog-digital converter (Digidata 1440A; Axon Instruments)18,56. Fluorescence intensities data were acquired using Clampex software (Axon Instruments). During measurements, cells were maintained in imaging buffer; 5 mM of 2,3-dimercapto-1-propanol (also called British anti-Lewisite—BAL) was added to the cells approximately 40 s after the recording started. Recovery of ECFP fluorescence was monitored over time and FRET efficiency was calculated as described here18,57. One independent experiment represents approximately 4–6 repeats (i.e. single-cell FRET signals) for each condition.
Peptide array and other peptide reagents
The peptide library comprised of peptides (13-mer peptides, 10 residue-overlap) with sequences derived from the IDRs of DVL3. This peptide library comprised a set of non-phosphorylated peptides and a set of phosphorylated peptides, in which the phospho groups were located at those residues corresponding to the previously identified CK1ε’s phosphorylation pattern29 (Supplementary Fig. 3). The designed peptide library was generated by JPT Peptide Technologies GmbH (Berlin, Germany) in an array format, wherein the peptides were immobilized on a glass slide.
In each experiment, two glass slides were used: one was as blank and another was screened with the recombinant CK1ε. Both slides were blocked by treatment with SmartBlock solution (Candor Bioscience, #113125) for 1 h at 30 °C. Then, one slide was incubated overnight with 10 μg/ml of the recombinant human CK1ε (MyBioSource, #MBS964562) in SmartBlock solution at 4 °C and the second one with SmartBlock solution only. The next day, both slides were washed in TBS buffer (4 × 10 min, RT) and then incubated with 1 μg/ml of the primary anti-CK1 antibody in SmartBlock solution for 1 h at 30 °C. The slides were subsequently washed again in TBS buffer (4 × 10 min, RT), followed by incubation with 1 μg/ml of secondary fluorescent antibodies in SmartBlock solution for 45 min at 30 °C, and subsequent washing in TBS buffer (4 × 10 min, RT) and in water (4 × 10 min, RT). To remove the excess of water, the slides were spinned down using a swing rotor (1200 r.c.f. for 2 min, RT, slides placed in 50 ml falcons). Binding of CK1ε to the peptides was detected by reading the fluorescence intensity of the peptide spots. In these experiments, the primary anti-CK1ε antibodies used were from Santa Cruz Biotechnology (#sc-6471) and from BD Biosciences (#610445), and the secondary antibodies used were: Alexa Fluor 594 Goat Anti-Mouse IgG2a (γ2a) (Invitrogen, #A-21135) and Alexa Fluor 594 Donkey Anti-Goat IgG (H + L) (Invitrogen, #A-11058). The slide data were analyzed using the PepSlide Analyzer software (Sicasys).
In each experiment, the signal intensity from each peptide on the experimental set of two slides (i.e. the one used as blank and the one screened with CK1ε) was normalized to 0–100%, where the 100% value corresponded to the strongest signal detected for one of the peptide spots within the CK1ε-screened slide. The intensities measured for the peptide spots on the control slide—which was incubated with the detection antibodies only—were then subtracted from the intensities measured for the corresponding peptide spots on the CK1ε-screened slide. Each experiment was repeated 2–3 times (2–3 technical replicates per experiment) using the same anti-CK1ε antibody and average values for each antibody were added up and plotted in the graph. The signals with the highest intensity involving at least four consecutive peptides were considered as a putative CK1ε-binding site. The signals shown in the graph (Fig. 3b) correspond to the non-phosphorylated peptides and their numbering is arbitrary.
The peptides used in the fluorescent polarization (FA) binding assays were synthesized at Pepscan B.V. (Lelystad, Netherlands). The sequences of these peptides (indicated in Supplementary Fig. 4a) were amidated at their C-termini, and their N-termini were acylated with 6-aminocaproic acid (Ahx) modified with fluorescein isothiocyanate (FITC). The peptides used in the NMR/SPR studies were purchased from KareBay Biochem, Inc. (New Jersey, USA). The peptides for the NMR/SPR studies contained no terminal modifications.
Data were recorded at 37 °C using Tecan Infinite F500 (Tecan Systems, Germany). FITC-labeled peptides were dissolved in DMSO and added to 384-well plates (Corning) to a total volume of 20 μl (peptide final concentration was 50 nM). Incubation with recombinant His-tagged human CK1ε (MyBioSource, #MBS964562) was performed for 30 min at 37 °C. Then, fluorescence intensities were collected simultaneously by detection at 535/590 and 485/535 nm excitation/emission wavelengths, respectively, followed by adjustment to the blank controls.
Samples were loaded onto SDS-PAGE gels, separated, and fixed with acetic acid in methanol, stained with Coomasie brilliant blue for 1 h and partially destained. Corresponding 1-D bands were excised. After destaining, the proteins in gel pieces were incubated with 10 mM DTT at 56 °C for 45 min. After removal of DTT excess samples were incubated with 55 mM IAA at room temperature in darkness for 30 min, then alkylation solution was removed, and gel pieces were hydrated for 45 min at 4 °C in digestion solution (5 ng/µl trypsin, sequencing grade, Promega, Fitchburg, Wisconsin, USA, in 25 mM AB). The trypsin digestion proceeded for 2 h at 37 °C on Thermomixer (750 r.p.m.; Eppendorf, Hamburg, Germany). Subsequently, the tryptic digests were subsequently cleaved by chymotrypsin (5 ng/µl, sequencing grade, Roche, Basel, Switzerland, in 25 mM AB) for 2 h at 37 °C. Digested peptides were extracted from gels using 50% ACN solution with 2.5% formic acid and concentrated in a speedVac concentrator (Eppendorf, Hamburg, Germany). The aliquot (1/10) of concentrated sample was transferred to LC-MS vial with already added polyethylene glycol (PEG; final concentration 0.001%)58 and directly analyzed by LC-MS/MS for protein identification.
The rest of the sample was used for phosphopeptide analysis. Sample was diluted with acidified acetonitrile solution (80% ACN, 2% FA). Phosphopeptides were enriched using Pierce Magnetic Titanium Dioxide Phosphopeptide Enrichment Kit (Thermo Scientific, Waltham, Massachusetts, USA) according to the manufacturer's protocol and eluted into LC-MS vial with already added PEG (final concentration 0.001%). Eluates were concentrated under vacuum and then dissolved in water and 0.6 μl of 5% FA to get 12 μl of peptide solution before LC-MS/MS analysis.
LC-MS/MS analyses of peptide mixture were done using the RSLCnano system connected to an Orbitrap Elite hybrid spectrometer (Thermo Fisher Scientific) with ABIRD (Active Background Ion Reduction Device; ESI Source Solutions) and Digital PicoView 550 (New Objective) ion source (tip rinsing by 50% acetonitrile with 0.1% formic acid) installed. Prior to LC separation, tryptic digests were online concentrated and desalted using trapping column (100 μm × 30 mm) filled with 3.5-μm X-Bridge BEH 130 C18 sorbent (Waters). After washing of trapping column with 0.1% FA, the peptides were eluted (flow 300 nl/min) from the trapping column onto Acclaim Pepmap100 C18 column (3 µm particles, 75 μm × 500 mm; Thermo Fisher Scientific) by 65 min long gradient. Mobile phase A (0.1% FA in water) and mobile phase B (0.1% FA in 80% acetonitrile) were used in both cases. The gradient elution started at 1% of mobile phase B and increased from 1% to 56% during the first 50 min (30% in the 35th and 56% in 50th min), then increased linearly to 80% of mobile phase B in the next 5 min and remained at this state for the next 10 min. Equilibration of the trapping column and the column was done prior to sample injection to sample loop. The analytical column outlet was directly connected to the Digital PicoView 550 ion source.
MS data were acquired in a data-dependent strategy selecting up to top six precursors based on precursor abundance in the survey scan (350–2000 m/z). The resolution of the survey scan was 60,000 (400 m/z) with a target value of 1 × 106 ions, one microscan, and maximum injection time of 200 ms. High-resolution (resolution 15,000 at 400 m/z) HCD MS/MS spectra were acquired with a target value of 50,000. Normalized collision energy was 32% for HCD spectra. The maximum injection time for MS/MS was 500 ms. Dynamic exclusion was enabled for 45 s after one MS/MS spectra acquisition and early expiration was disabled. The isolation window for MS/MS fragmentation was set to 2 m/z.
The analysis of the mass spectrometric RAW data files was carried out using the Proteome Discoverer software (Thermo Fisher Scientific; version 1.4) with in-house Mascot (Matrixscience; version 2.4.1) search engine utilization. MS/MS ion searches were done against in-house database containing expected protein of interest with additional sequences from cRAP database (downloaded from http://www.thegpm.org/crap/). Mass tolerance for peptides and MS/MS fragments were 7 ppm and 0.03 Da, respectively. Oxidation of methionine, deamidation (N, Q), and phosphorylation (S, T, Y) as optional modification, carbamidomethylation of C as fixed modification, and three enzyme miss cleavages were set for all searches. The phosphoRS feature was used for phosphorylation localization.
Quantitative information was assessed and manually validated in Skyline software (Skyline daily 220.127.116.1184).
Numerical data and statistics
As for numerical data, mean ± S.D. (or median ± interquartile range, respectively) are shown as depicted. No pairing one-way ANOVA test with Gaussian distribution (with Tukey's post-test) was used for comparison of more than two samples; for two-column statistics in Figs. 3e, g and 5b, unpaired two-tailed Student's t-test was used (*, p ≤ 0.05; **, p ≤ 0.01; ***, p ≤ 0.001, ****, p ≤ 0.0001; ns, not significant, p > 0.05).
Data on frequency of puncta vs. even (Fig. 8b) were analyzed using Generalized Linear Mixed Model (GLMM) with binomial distribution of dependent variable, treatment as fixed effect, and experiment as random effect variable, since data within the experiments are not independent. In case of evaluation of DVL-membrane recruitment results (Fig. 8c), the GLMM with multinomial distribution was used. Results were presented as odds ratios (OR) with 95% confidence intervals. Data were analyzed in R software. All numerical data were analyzed by MS Excel 2007 and arranged in the graphs using GraphPad Prism 6 software.
Multiple sequence alignment
The multiple sequence alignment of selected sequences was performed by ClustalW algorithm. Output alignment was refined manually using the BioEdit v7.0.1 sequence editor.
Protein expression and purification
The PDZ domain of human DVL2 wild type (aa 265–361) and phosphorylation-mimicking variant S286E + S329E were cloned into pET vector containing an N-terminal His6-tag and a lipoyl domain separated by a Tobacco Etch Virus (TEV) protease digestion site from the N-terminus of the inserts. Both proteins were expressed at high yields in E. coli BL21 (DE3) strain (New England Biolabs, #C2527I). For the NMR studies, 13C- and 15N-labeled proteins were prepared by growing cells in minimal medium supplemented with 15NH4Cl (1 g/l) and 13C6 glucose (2 g/l) as the sole nitrogen and carbon sources, respectively. Cells were grown at 37 °C to an OD600 of approximately 0.8 and protein expression was induced with 0.5 mM IPTG. Cells were lysed by sonication and centrifuged at 15,000g. Three purification steps were used for both proteins: Ni-NTA chromatography followed by overnight TEV cleavage to remove the N-terminal His6-tag and the lipoyl domain, ion exchange chromatography, and size exclusion chromatography. Finally, the untagged PDZ domain wild type or phosphorylation-mimicking variant was concentrated and exchanged to buffer for NMR or binding experiments containing 20 mM HEPES (pH 6.8) and 50 mM KCl. Human CK1ε (aa 1–294) was also cloned into a pET vector and purified using three purification steps as described for the PDZ domain.
Full-length DVL3 used as a substrate in the kinase assay was produced as follows: Twin-Strep-tag N-terminally tagged DVL3 was expressed in HEK293 cells using transient transfection. Cells were harvested 48 h post-transfection, resuspended in a lysis buffer (50 mM Tris, 150 mM NaCl, 10 mM KCl, 10% glycerol, pH 8) with cocktail of protease inhibitors (#11836145001, Roche) and 0.2% NP40 (#74385, Sigma). The mixture was incubated for 20 min on ice and cell lysis was enhanced by sonication. Cell lysate was cleared by centrifugation at 100,000g for 45 min at 4 °C and supernatant was loaded on Strep-Tactin Superflow high capacity column (#2-1237-001, IBA) equilibrated in the lysis buffer. The column was washed in lysis buffer and the protein was eluted using lysis buffer supplemented with 3 mM desthiobiotin. Eluted proteins were concentrated to 1 mg/ml using protein concentrators (#88516; Thermo Fisher Scientific), flash frozen in liquid nitrogen, and aliquots were stored at −80 °C.
In vitro kinase assay
Full-length DVL3 protein and CK1ε kinase were dialyzed into phosphorylation buffer (50 mM sodium phosphate, pH 6.5, 50 mM KCl, 10 mM MgCl2, 1 mM DTT, 1 mM EDTA). In each reaction, DVL3 and CK1ε were mixed in 2:1 ratio (containing ~0.5 μM DVL3, ~0.25 μM CK1ε kinase, and 1 mM ATP), and incubated at 25 °C for 16 h. Samples were subsequently analyzed by SDS-PAGE and mass spectrometry.
A 4D HC(CC-TOCSY(CO))NH and a 4D 13C, 15N edited HMQC-NOESY-HSQC experiments were recorded at CEITEC Josef Dadok National NMR Centre on a 700 MHz Bruker Avance III spectrometers equipped with 1H/13C/15N TCI cryogenic probe head with z-axis gradients. 4D spectra were processed with SSA package59 and analyzed with SPARKY. Chemical shift assignments were obtained automatically using 4D-CHAINS60 and checked manually. NMR titrations were performed in series of 1H, 15N HSQC spectra using 100 μM of 15N-labeled protein (wild type or phosphorylation-mimicking variant) and increasing amounts of C-terminal DVL peptide (pS700) consisted of aa 698–716 from DVL3 (stock concentration of 800 μM). Steady-state15N-1H Nuclear Overhauser Effect values were measured under a steady-state condition with a 30 s interscan relaxation delay. Reference spectra and the spectra measured under steady-state conditions were measured in an interleaved manner.
Surface plasmon resonance
SPR experiments were performed on a Biacore T200 instrument (GE Healthare). The wild type and phosphorylation-mimicking variant of PDZ from DVL2 were immobilized on carboxy-methylated dextran matrix (CM5 chip S Series) using amino coupling. Non-reacted groups were blocked by 1 M ethanolamine. The blank channel was modified by NHS/EDC activation and subsequently blocked by ethanolamine. The C-terminal DVL peptide (aa 698–716 from DVL3; pS700) was injected at increasing concentrations and long enough to reach steady state. SPR responses were measured and corrected for the response of the blank. Data points were collected from each binding sensogram before the end of the injection (equilibrium) and the dissociation constants were estimated by fitting the response at equilibrium versus the C-terminal peptide concentration using the following equation: Req = C*Rmax/(KD + C), where Req is the binding level in Response Units at different C-terminal peptide concentrations (C), Rmax the response at saturation (fitted), and KD the apparent dissociation constant (fitted).
In silico simulation methodology
All simulations were done in Gromacs 5.1.2 simulation package61. Each simulation contained a PDZ domain in a salt solution of 150 mM NaCl. The initial structure of wild-type PDZ domain (aa 245–338) from DVL3 was constructed by homology modeling using MODELLER v9.11 (refs. 62,63). As a template we used crystal structure of human DVL2 (PDB ID: 2REY) which share 96.28% sequence identity. Missing loops and one missing residue at C-terminus were added via MODELLER64. Quality of seven generated models was evaluated based on DOPE and GA341 score and the best structure has been selected for further use in molecular dynamics. Mutation of serine residues S268 and S311 to either glutamic acid (E) or phosphoserine were done with MODELLER. The initial structure of C-terminal peptide bound to PDZ domain was taken from the Coarse-Grained simulation using PLUM parameterization65, where a position of the C-terminal peptide was sampled around the whole PDZ domain and most probable configuration was chosen as a starting structure.
We employed all-atom force field amber99sb-ILDN66 with phosphoserine parameters67 in explicit TIP3P68 water model. Robert Best’s correction for disordered proteins/regions was applied by scaling van der Waals interactions between water oxygen and protein with factor 1.1 (ref. 69). All systems were solvated in ~10,000 water molecules placed in a cubic box, where the protein is surrounded by at least 1.3 nm from the box side. Protonation state of all residues was chosen according to neutral pH = 7 with histidine H324 neutral. If not stated otherwise, all proteins were capped at C-terminus by an acetyl group and at N-terminus by N-methyl to remove artificial charge introduced at protein ends.
All simulations were performed for at least 300 ns with 2 fs time step. The systems were kept in NPT ensemble at 309.15 K. Temperature was controlled using a velocity-rescaling thermostat70 with a coupling constant of 0.1 ps applied separately to solvent and protein. The pressure was hold at 1 bar via an isotropic Parrinello–Rahman barostat71,72, with coupling time 2 ps. Cut-off distance for direct space electrostatic and van der Waals interactions was set to 1 nm. Long-range electrostatic contribution was evaluated by using the particle-mesh Ewald summation method73,74, with a maximal distance between FFT grid points of 0.12 nm and fourth interpolation order. All covalent bonds of hydrogen atoms were constrained with LINCS algorithm75. All systems were simulated using periodic boundary conditions.
The mean enthalpic energy contribution for each amino acid pair was calculated from the sum of the Lennard–Jones and Coulombic contributions for the whole residue including both backbone and side-chain atoms. Averages were taken from the whole 500 ns long production dynamics.
Further information on experimental design is available in the Nature Research Reporting Summary linked to this article.
Data supporting the findings of this manuscript are available from the corresponding author upon reasonable request. A reporting summary for this article is available as a Supplementary Information file. The source data underlying Figs. 1d, 2a, c, d, 3e, g–h, j, 4a, c, d, 5b–e, 6h, j, 7e, f, 8b–d and Supplementary Figs 1c, e, 2a, b, 4a–d, f, 7b are provided as a Source Data file. The mass spectrometry proteomics data have been deposited to the ProteomeXchange Consortium via the PRIDE76 partner repository with the dataset identifier PXD013085. Figures were deposited in figshare depository possessing the identifier DOI 10.6084/m9.figshare.7856168
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We would like to thank Lucie Nesvadbová, Lenka Bryjová, Pavlína Žofka Mrhálková, and Naďa Bílá for excellent assistance, and the members of the Bryja Lab for helpful discussions. Also, we would like to thank Petra Ovesná for help with the statistics in Fig. 8. Special thanks go to Kathyann Lee for the help with English Language editing and review. The work was supported by Czech Science Foundation (project no. GA15-21789S, GA18-17658S, and GA19-26041x), Grant Agency of Masaryk University (MUNI/G/1100/2016, MUNI/G/0739/2017, MUNI/E/0533/2018). J.H. specially thanks for the support of the EMBO Short-Term Fellowship (no. ASTF 687-2016). Furthermore, this research was supported by project CEITEC 2020 (no. LQ1601) with financial contribution from the MEYS CR and National Programme for Sustainability II to R.V., M.J., K.T., L.T., K.H. and J.R. and by the; project SYMBIT (CZ.02.1.01/0.0/0.0/15_003/0000477) funded by the European Regional Development Fund and by the MEYS CR; CIISB research infrastructure project LM2015043 funded by MEYS CR is gratefully acknowledged for the financial support of the measurements at CEITEC Josef Dadok National NMR Centre and Proteomics Core Facility. J.R. thanks for support of Ministry of Health of the Czech Republic project (no. 15-34405A). M.C.A.C. and C. Hoffmann were supported by the ITN WntsApp (grant no. 608180; www.wntsapp.eu) and the Deutsche Forschungs-gemeinschaft (DFG, German Research Foundation)—TRR166: project C2. Computational resources were provided by the CESNET LM2015042 and the CERIT Scientific Cloud LM2015085 provided under the program “Projects of Large Research, Development, and Innovations Infrastructures”. This work was supported from European Structural and Investment Funds, Operational Programme Research,Development and Education – "Preclinical Progression of New Organic Compounds with Targeted Biological Activity” (Preclinprogress) -CZ.02.1.01/0.0/0.0/16_025/0007381. Additional computational resources were obtained from ‘IT4 Innovations National Supercomputing Center -- LM2015070’ project supported by MEYS CR from the Large Infrastructures for Research, Experimental Development and Innovations. C. Holler and A.S. were supported by Deutsche Forschungsgemeinschaft (DFG, German Research Foundation), grant SCHA965/6-2.
The authors declare no competing interests.
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Harnoš, J., Cañizal, M.C.A., Jurásek, M. et al. Dishevelled-3 conformation dynamics analyzed by FRET-based biosensors reveals a key role of casein kinase 1. Nat Commun 10, 1804 (2019). https://doi.org/10.1038/s41467-019-09651-7
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