Facilitation of axon outgrowth via a Wnt5a-CaMKK-CaMKIα pathway during neuronal polarization
- Shin-ichiro Horigane†1, 2,
- Natsumi Ageta-Ishihara†1, 3,
- Satoshi Kamijo1, 4,
- Hajime Fujii1, 4,
- Michiko Okamura1,
- Makoto Kinoshita3,
- Sayaka Takemoto-Kimura1, 2, 5Email author and
- Haruhiko Bito1, 4Email author
© Horigane et al. 2016
Received: 3 December 2015
Accepted: 10 January 2016
Published: 16 January 2016
Wnt5a, originally identified as a guidance cue for commissural axons, activates a non-canonical pathway critical for cortical axonal morphogenesis. The molecular signaling cascade underlying this event remains obscure.
Through Ca2+ imaging in acute embryonic cortical slices, we tested if radially migrating cortical excitatory neurons that already bore primitive axons were sensitive to Wnt5a. While Wnt5a only evoked brief Ca2+ transients in immature neurons present in the intermediate zone (IZ), Wnt5a-induced Ca2+ oscillations were sustained in neurons that migrated out to the cortical plate (CP). We wondered whether this early Wnt5a-Ca2+ signaling during neuronal polarization has a morphogenetic consequence. During transition from round to polarized shape, Wnt5a administration to immature cultured cortical neurons specifically promoted axonal, but not dendritic, outgrowth. Pharmacological and genetic inhibition of the CaMKK-CaMKIα pathway abolished Wnt5a-induced axonal elongation, and rescue of CaMKIα in CaMKIα-knockdown neurons restored Wnt5a-mediated axon outgrowth.
This study suggests that Wnt5a activates Ca2+ signaling during a neuronal morphogenetic time window when axon outgrowth is critically facilitated. Furthermore, the CaMKK-CaMKIα cascade is required for the axonal growth effect of Wnt5a during neuronal polarization.
KeywordsWnt5a Axon outgrowth Ca2+ signaling CaMKIα CaMKK
The formation of functional neuronal circuits requires a combination of a cell’s intrinsic genetic program and extracellular factors . Wnt proteins are highly conserved, secreted morphogens that activate the β-catenin-mediated canonical pathway as well as planar cell polarity and Ca2+-mediated non-canonical signaling pathways [2, 3]. In addition to their primary functions during the early developmental stages, Wnt proteins have been shown to regulate the cerebral cortex throughout development during various morphogenetic processes, such as anterior–posterior axis formation, neural patterning, radial migration, development of neurites (axon and dendrites), and formation of dendritic spines, both in culture and in vivo. These data indicate that Wnt signaling may play a crucial role throughout the development of the neuronal circuits [4, 5].
One of the most extensively studied Wnt proteins is Wnt5a. Wnt5a activates a non-canonical Wnt pathway that is conserved from Caenorhabditis elegans to humans and regulates a variety of cellular functions . In the central nervous system, an unexpected role for Wnt5a and its receptor Derailed/Ryk in axon guidance has been reported in drosophila  and in mice [8, 9]. A gradient of Wnt5a expression has been proposed to induce the repulsion of axons in the corticospinal tract  and cultured neurons , as well as in cortical slices . Paradoxically, and concurrent with this repellant activity, Wnt5a facilitated axonal outgrowth by increasing the rate of outgrowth . Previous pharmacological studies have indicated that Wnt5a might activate Ca2+/calmodulin-dependent kinase II (CaMKII), resulting in axonal outgrowth and turning by cortical neurons [11, 12]. Furthermore, Wnt5a was also implicated in activation of PKC through a Ca2+ pathway that causes the axonal branching and elongation of sympathetic neurons . Collectively, these studies suggested an important role for Wnt5a-activated Ca2+ signaling during axonal morphogenesis of several neuronal cell types.
Recent research has drawn attention to the activity of CaMKI, a distinct branch of the CaMK family, during Ca2+-dependent neuronal morphogenesis. CaMKI has 4 isoforms: α, β/Pnck, γ/CL3, δ/CKLiK [14–17], all of which share the requirement for both Ca2+/calmodulin and an upstream kinases CaMK kinase α (CaMKKα) or CaMKKβ [18–20]. Our previous studies had shown that CaMKIα facilitated axonal elongation through GABA-dependent Ca2+ elevation , while CaMKIγ promoted dendritic outgrowth through BDNF-mediated Ca2+ elevation . Consistent with these results, inhibition of CaMKKα/β activity impaired outgrowth of both axons and dendrites in immature cortical neurons in culture .
Based on the above observations, we first sought to determine the time window during which Wnt5a-Ca2+ pathway may have a critical morphogenetic role. Combining Fluo-4 Ca2+ imaging and in utero electroporation in acute embryonic cortical slices, we tested if radially migrating cortical excitatory neurons that already bore primitive axons were sensitive to Wnt5a. While Wnt5a only evoked brief Ca2+ transients in immature neurons present in IZ, Wnt5a-induced Ca2+ oscillations were sustained in neurons that migrated out to CP. This raised the possibility that early Wnt5a-Ca2+ signaling during neuronal polarization has a morphogenetic consequence. Consistent with this idea, administration of Wnt5a induced axonal, but not dendritic, outgrowth in immature cortical neurons. Pharmacological and genetic inhibition of the CaMKK-CaMKI pathway abolished Wnt5a-mediated axonal elongation. Furthermore, the defective axonal growth during RNA interference against CaMKIα was rescued by a short hairpin RNA (shRNA)-resistant, wild-type CaMKIα. Collectively, our results demonstrate that CaMKK-CaMKIα is a major signaling cascade in Wnt5a-mediated axonal elongation, particularly during the early stages of neuronal polarization.
Activation of Wnt5a-Ca2+ signaling in radially migrating cortical neurons
Previous findings suggested a role for Wnt5a in driving Ca2+ signaling during growth of callosal axons [9, 11, 12], but whether Wnt5a acted on axonal outgrowth at an earlier stage of corticogenesis was not examined. We therefore tested whether Wnt5a administration could mobilize intracellular Ca2+ concentrations in radially migrating cortical neurons which had just begun to extend axons in vivo. During migration, excitatory neurons transit from a multipolar to a bipolar shape at the upper IZ and exit into CP. Through a morphogenetic process that occurs in parallel to the determination neuronal cell polarity, most neurons begin to grow axons in IZ and extend them while they radially migrate into CP towards the pial surface [1, 23]. Therefore, we focused our examination of Wnt5a-Ca2+ signaling on bipolar-shaped neurons that had just begun to extend a primitive axon and were located in IZ and CP.
Wnt5a stimulates elongation of axons but not dendrites in immature cultured cortical neurons
Our finding that Wnt5a-Ca2+ signaling was active in immature excitatory neurons that had just begun to extend axons in acute cortical slices was further confirmed by Ca2+ imaging experiments in immature cultured cortical neurons (Additional file 3: Figure S1, Additional file 4: Movie 3). These evidences prompted us to next investigate whether Wnt5a had a morphogenetic effect on immature cortical neurons during neuronal polarization.
Wnt5a promotes axonal elongation via a CaMKK-CaMK signaling cascade
Pharmacological studies carried out at a slightly later stages of culture have suggested that Wnt5a-Ca2+ signaling may be mediated by CaMKII, resulting in axon outgrowth and turning in cortical neurons [9, 11, 12]. An independent branch of Ca2+-dependent CaMK family comprises the CaMKI subfamily (α, β, γ, and δ), which may form several parallel kinase cascades downstream of CaMKKα and/or CaMKKβ. Recent reports, including ours, have begun to shed light on the essential role of CaMKI in the regulation of neuronal morphogenesis both in vitro and in vivo [20–22], such as promoting growth cone motility , neurite outgrowth [27–29], activity-dependent growth of dendrites [22, 30], and stabilization of spines . Based on these findings, we critically examined whether a CaMKK-CaMK cascade may play a role in Wnt5a-Ca2+ signaling during early axon outgrowth.
An essential role of CaMKIα in mediating axon-specific facilitation of outgrowth induced by Wnt5a during neuronal polarization
Taken together, these results provide evidence for a significant role of a CaMKK-CaMKIα cascade in mediating the facilitatory effects of Wnt5a on axon elongation during neuronal polarization. Furthermore, our findings suggest that CaMKIα may be a common axonogenic effector which mediates the effects of multiple Ca2+ response-inducing extracellular morphogens, such as excitatory GABA and Wnt5a.
In this study, we have explored a new role for Wnt5a-Ca2+ signaling in a very early stage of cortical morphogenesis and found that even immature migrating neurons, which just entered CP and bore only primitive axons, were already responsive to Wnt5a and capable of activating a Ca2+ -triggered pathway. Though the majority of studies on the in vivo effects of Wnt5a hitherto have focused on the development of commissural axons, such as those in the spinal cord and corpus callosum, our findings are consistent with a significant expression of Wnt5a mRNA in the embryonic CP , where immature neurons dramatically alter their shape by extending axons vertically in a direction opposite to their radial migration. While our study suggest a Ca2+-basis for Wnt5a-mediated control of axon growth, perhaps through facilitation of its repulsive activity , future studies are needed to clarify whether Wnt5a is indeed released from CP neurons and whether such ambient Wnt5a may form a gradient akin to that previously proposed in the corpus callosum surrounding commissural axons.
In keeping with our discovery of early time window of Wnt5a sensitivity in immature cortical neurons, an increase in Wnt5a signaling was recently reported to suppress canonical Wnt/β-catenin signaling, thus underlying a critical permissive role for Wnt5a during multipolar-to-bipolar morphological transition . Furthermore, it has been suggested that Wnt5a proteins guide cell morphogenesis that accompanies cell migration in a variety of cellular systems [6, 41]. Thus, Wnt5a-Ca2+ signaling might facilitate and coordinate two cellular processes in newly bipolar shaped neurons—directional movement and axonal outgrowth, both of which are critical for proper corticogenesis.
Capitalizing on our own previous findings that a CaMKK-CaMKIα cascade might have a potent and selective axonogenic activity , we here have specifically investigated whether Wnt5a had a selective growth promoting effect on axons, and if so, whether a part of this might be mediated by a Ca2+-dependent CaMKK-CaMKIα pathway. Results from pharmacological, knockout and knockdown experiments unequivocally demonstrated a strong involvement of CaMKKs and CaMKIα in Wnt5a-faciliated axonal outgrowth. A recent study revealed that Wnt5a induced membrane insertion and clustering of functional GABAA receptors that increased the amplitude of GABA currents in adult hippocampal neurons . If such a mechanism were conserved in immature cortical neurons, one might imagine that direct Wnt5a effects might synergize with those of an indirect, depolarizing GABAA-mediated Ca2+ signaling in immature neurons. Alternatively, Wnt5a and GABAA pathways might cooperate to evoke a common downstream Ca2+ signaling leading to ultimate activation of the CaMKK-CaMKIα pathway. Either way, our results indicate that CaMKIα activation would be a likely common Ca2+ pathway downstream of a versatile mixture of extracellular ligands. How this event then leads to phosphorylation of key substrates that modulate of cytoskeletal remodeling and membrane trafficking and trigger selective neuritic growth is currently under investigation [20, 43].
This study suggests that Wnt5a activates Ca2+ signaling during a neuronal morphogenetic time window when axon outgrowth is critically facilitated. Furthermore, the CaMKK-CaMKIα cascade is required for the axonal growth effect of Wnt5a during neuronal polarization. These results support the notion that the CaMKIα pathway underlies axonal development in response to a wide variety of extracellular signaling molecules that are necessary to achieve precise cortical wiring.
All recombinant DNA and animal experiments in this study were performed in accordance with regulations and guidelines for the care and use of experimental animals of the University of Tokyo and were approved by the institutional review committees of the University of the Tokyo Graduate School of Medicine.
In utero electroporation
In utero electroporation (IUE) was performed for labeling radially migrating neurons as described previously [21, 24]. In brief, pregnant ICR mice at E14.5 or E15.5 were deeply anesthetized with Pentobarbital Sodium, and 2.0 μg/μl plasmid solution colored with Fast Green (0.1 %) was injected into the lateral ventricle of the mouse embryos through glass capillaries (GC150TF-10, Harvard Apparatus) pulled by a micropipette puller. Electroporation (5 pulses of 45 V, 50 ms) was then applied using an electroporator (ECM 830, BTX) with a tweezer-type electrode (CUY650P5, BEX Co. Ltd).
Preparation of cortical slices
Brains were quickly removed from mice embryos 65–70 h after IUE, at E17.5, and embedded in 3 % low-melting temperature agarose (SeaPlaque Agarose, Lonza) dissolved in a solution containing: (in mM) 27 NaHCO3, 1.4 NaH2PO4, 2.5 KCl, 0.5 ascorbic acid, 7.0 MgSO4, 1.0 CaCl2, and 222.1 sucrose . Then, each mouse brain was immersed in this ice-cold solution bubbled with a gas mixture of 95 % O2 and 5 % CO2, and 300 μm-thick coronal slices were prepared using a vibratome (VT1000, Leica). After preparation, the slices were recovered for over 30 min at room temperature in an artificial cerebrospinal fluid (aCSF) consisting of: (in mM) 127 NaCl, 26 NaHCO3, 1.5 KCl, 1.24 KH2PO4, 1.4 MgSO4, 2.4 CaCl2, and 10 glucose .
Fluo-4 AM loading into cortical slices
In order to load Fluo-4 AM (Invitrogen), cortical slices were transferred to 35-mm dishes filled with a solution containing Fluo-4 AM (10 μM Fluo-4 AM, 0.01 % Pluronic F-127, and 0.005 % Cremophor EL were dissolved in aCSF), and incubated for 30 min at 37 °C and 5 % CO2 in a microincubator (Tokai Hit). After washing, the slices were maintained in a Fluo-4-free aCSF solution at room temperature for at least 30 min.
Ca2+ imaging analyses
After Fluo-4 AM loading, cortical slices were transferred to a perfusion chamber (RC-22, Harvard Apparatus) attached to a LSM510META confocal laser microscopy system (Carl Zeiss) and perfused with physiological aCSF containing: (in mM) 127 NaCl, 26 NaHCO3, 3.3 KCl, 1.24 KH2PO4, 1.0 MgSO4, 1.0 CaCl2, and 10 glucose [44, 45] bubbled with 95 % O2 and 5 % CO2 at 37C°. Time-lapse Fluo-4 and TagRFP images were acquired sequentially using an oil-immersion objective (Plan-Neofluar 40×/1.30NA, Carl Zeiss) and Multi-track mode of data collection software (Zen, Carl Zeiss) at 0.5 fps with 512 × 512 pixels. Fluo-4 and TagRFP were excited by Argon (488 nm) and HeNe (543 nm) laser lines, and their emission signals were selected by 505-550 band-pass filter and 561-615 spectral imaging detector, respectively. After baseline imaging, aCSF containing 10× Wnt5a (1× final concentration: 100 nM) was gently bath-applied. Fluorescence signals in the cell bodies of individual migrating neurons, identified by TagRFP expression, were quantified using Image J software.
To correct for motion and focusing artifacts during the imaging of migrating neurons, we normalized Fluo-4 fluorescence intensity against the fluorescence of the volume-filling TagRFP. Briefly, we calculated F(TagRFP)/F0(TagRFP) from the fluorescent intensity of TagRFP after background subtraction, where F0(TagRFP) is the averaged intensity of all imaging periods, and F(TagRFP) is the fluorescence intensity at any time point. Finally, ΔF/F0, expressed as a percentage, was calculated as (ΔF(Fluo ‐ 4)/F0(Fluo ‐ 4))/ (F(TagRFP)/F0(TagRFP)).
For Ca2+ imaging of immature cultured cortical neurons, a G-CaMP7-based Ca2+ indicator  and S.K. et al. in preparation was expressed in cortical layer 2/3 neurons by IUE of ICR mice at E15.5, and expressing hemispheres were collected at E18.5. Following mild trypsin digestion and gentle mechanical trituration, 2.0 × 105 dissociated neurons were plated onto poly-D-lysine coated glass bottom dishes (MatTek) and maintained for two days in minimal essential medium (MEM) supplemented with 10 % fetal bovine serum (FBS) and with 2 % NS21 . All imaging experiments were performed at 37 C° and 5 % CO2 in a stage top incubator (Tokai Hit) mounted on an IX71 microscope (Olympus). The images were acquired at 256 × 256 pixels using an oil-immersion lens (60×/1.49NA) and a C9100-12 EM-CCD (Hamamatsu Photonics) at 1fps with an exposure time of 100 ms. We used FF01-474/23, FF02-520/28 filters (Semrock) as excitation and emission filters respectively. The excitation light was supplied by a Lambda-DG4 (Sutter Instruments) Xenon lamp light source. During imaging, 5 × concentrated Wnt5a-containing culture medium (500 ng/ml) was manually added to the imaging dish with a syringe.
Preparation of primary cortical cultures for morphometric analysis
Primary cultures of immature cortical neurons were prepared from embryonic day 19 (E19) Sprague-Dawley rats or E17 C57BL/6 mice (wild-type and DKO mutant mice) were prepared as previously described . In brief, after dissection, cortices were incubated for 10 min with 10 mg/ml trypsin type XI (Sigma-Aldrich) plus 0.5 mg/ml DNase I type IV (Sigma-Aldrich) at room temperature and mechanically dissociated in Hanks’ solution, pH 7.4 (Sigma-Aldrich), with 0.5 mg/ml DNase I type IV and 12 mM MgSO4. Dissociated neurons were transfected by electroporation using Nucleofector (Amaxa Biosystems) and plated onto either poly-L-lysine-coated 12 mm coverslips (BD Biosciences), poly-D-lysine-coated glass-bottom dishes (MatTek), or six-well dishes (BD Biosciences), and cultivated in minimum essential medium (Invitrogen) containing 5 g/L glucose, 0.2 g/L NaHCO3, 0.1 g/L transferrin (Calbiochem), 2 mM GlutaMAX-I (Invitrogen), 25 μg/ml insulin (Sigma-Aldrich), B-27 supplement (Invitrogen), and 10 % fetal bovine serum. All primary cortical cultures were incubated in 5 % CO2 at 37 °C.
Pharmacological stimulation and inhibition experiments
Wnt5a (R&D Systems), KN-93 (Calbiochem), or STO-609 (Tocris Bioscience) were applied to the medium of cultured cortical neurons expressing mRFP1 for morphometric analysis from 6 h after plating onwards . Final drug concentrations were 400 ng/ml (Wnt5a), 10 μM (KN-93), or 2.6 μM (STO-609). Bath application was performed by dissolving the reagents in one-half volume of the conditioned culture medium and then mixing this volume gently with the remaining volume of the original medium that remained in the dish. The culture medium was not changed before fixation.
Construction of shCaMKIα vector and shRNA-resistant wild-type CaMKIα vector
For RNAi experiments, a shCaMKIα vector co-expressing mRFP1 as a morphological tracer was constructed essentially as described . In brief, to create pSUPER-shCaMKIα complementary 60-bp oligonucleotides carrying antisense and sense sequences for CATTGTAGCCCTGGATGAC (19-bp, corresponding to nucleotides 231–249 of mouse CaMKIα) were subcloned into the pSuper + mRFP1 plasmid backbone. pSUPER-shNega was generated similarly, except that an artificial 19-mer sequence (ATCCGCGCGATAGTACGTA) was used as a target . This sequence was based on a commercially available negative control siRNA sequence (B-Bridge International) that we confirmed had no significant similarity to any known mammalian gene using the Basic Local Alignment Search Tool (BLAST). For generating the shCaMKIα-resistant construct, silencing mutations were introduced into the shCaMKIα target sequence of rat wildtype CaMKIα cDNAs , and the mutated rat CaMKIα cDNA was inserted into the pEGFPC1 vector (BD Clontech).
Generation of the CaMKKα/β-DKO mouse line
CaMKKα-KO mice have been described previously , and CaMKKβ-KO mice were previously created [21, 49]. In brief, similar to CaMKKα-KO mice, exon 2 (harboring the ATG start codon) through exon 6 of the CaMKKβ gene was deleted in CaMKKβ-KO mice. A detailed characterization of the CaMKKβ-KO mice has been published . CaMKKα-KO and CaMKKβ-KO mice were crossed to produce a CaMKKα/β-double knockout (DKO) mouse line. The DKO line and wild type C57BL/6 mice were crossed to produce a CaMKKα/β-double heterozygous (DHT) mouse line as a control.
Quantitative analysis of axons and dendrites
For quantification of process length and tip number, cortical cultures were transfected with plasmids encoding CAG promoter-driven mRFP1 by electroporation, plated onto 12-mm poly-L-Lysine-coated coverslips at the density of 5 × 105 cells (rats) or 7.5 × 105 cells (mice) per coverslip in 24-well plates, and then fixed at 2 Days In Vitro. Morphometric analyses were performed using immunofluorescence images of mRFP1 captured by an Olympus BX51 microscope system with a 20 × objective. Axons and dendrites were identified using standard morphological criteria and only neurons that exhibited one clearly classifiable axon and one or more dendrites were analyzed. For all quantitative analyses, the observer was blinded to the identity of the transfected constructs, mice genotypes, and drug treatments.
Statistical analyses were performed using Prism 4.0 (GraphPad Software). The student’s t-test was used for comparisons of the two groups. One- or two-way analysis of variance (ANOVA) with post-hoc Turkey-Kramer or Bonferroni test was used for factorial analysis between three or more groups. All data are reported as the mean ± standard error of mean (SEM).
We thank T.A. Chatila (Boston Children’s Hospital) for kindly providing access to CaMKKα and CaMKKβ KO mice. We thank K. Nakajima, T. Kawauchi (Keio Univ.), and Y.V. Nishimura (Doshisha Univ.) for technical help in initiating live imaging of migrating cortical neurons. This work was supported in part by grants from CREST-AMED (to H.B.), PRESTO-JST (to S.T.-K.), KAKENHI grants from JSPS (to N.A.-I., M.O., M.K., S.T.-K. and H.B.), and awards from Narishige Neuroscience Research Foundation, the Sumitomo Foundation, the Astellas Foundation for Research on Metabolic Disorders (to S.T.-K.), the Japan Foundation for Applied Enzymology (to H.B.) and the Takeda Science Foundation (to S.T.-K. and H. B.). We thank all members of the Takemoto and Bito laboratories for support and discussion. We are particularly indebted to Y. Kondo, K. Saiki, K. Gyobu, Y. Dobashi, Y. Tanabe, N. Shimada, M. Suzuki and T. Kinbara for assistance.
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