Collective cell migrations play key roles in gastrulation, organogenesis, wound healing, and immune responses, as well as pathological processes including chronic inflammation and cancer invasion1,2. Tissues undergo various types of collective cell migration. Epithelial cells, for example, have been observed to migrate in lines, sheets, strands, and hollow tubes. They rely on stable cell-cell junctions (especially adherens junctions) to maintain cooperativity. In contrast, migratory mesenchymal cells only have transient cell-cell contacts1,2. This could be problematic when the cell density is high or the migration distance is long (millimeter or centimeter range). Either situation greatly limits guidance cues available to cells at the rear of the migrating cohort2,3. Therefore, biological systems must have developed mechanisms to boost and relay directional signals.

Externally applied electric fields were found to guide directional migration of cultured cells4. Recent studies revealed that long-range, self-sustained K+ oscillations coordinate collective proliferation and migration in bacteria5,6. Endogenous direct-current (DC) electric fields (EFs) have also been detected during embryogenesis/regeneration in eukaryotes and these EFs were implicated in instructing cells with directional or positional information7,8,9,10. However, the molecular understanding of these phenomena is rudimentary, mainly due to a lack of tools to monitor endogenous electric fields with high spatiotemporal resolution in vivo. The development of tools such as vibrating probes11 and genetically encoded voltage- and Ca2+ sensors12,13 enables in-depth investigation of bioelectric signals in vivo.

Feather bud elongation in chicken dorsal skin explants is a very robust and precise biological process, even without the embryonic microenvironment14,15. The robustness of this process implies the maintenance of localized and stringent molecular mechanisms for coordinating collective cell behaviors. Previous studies of cellular events implicate polarized mesenchymal cell rearrangements in directed feather bud elongation16. Sparse BrdU- or TUNEL-positive cells in feather mesenchyme imply minimal involvement of cell divisions or apoptosis, a potentially confounding interpretation16,17. We hypothesize that tissue endogenous bioelectric signals mediated by ion channels, exchangers and pumps may carry out the signal relay function in mesenchymal cells during feather elongation.

In this study we observed dynamic changes of bioelectric currents in developing chicken embryos. Before feather bud elongation, EF endogenous to dorsal skin was relatively homogenous and exhibited inward directionality. At the onset of elongation, outward electric current emerged at the anterior side of each feather bud, implying a heterogenization of the EF into multiple smaller electric circuits. Tissue-wide long-range Ca2+ oscillations were observed in bud mesenchyme. Dampening these oscillations or introduction of exogenous oscillations altered feather morphology. Feather mesenchymal cell movement changes direction markedly when voltage-gated Ca2+ channels (VGCCs) or gap junctions were inhibited. The landscape of the Connexin-43 based gap junction network was modulated by synergistic actions of SHH and WNT signaling. This network electrically coupled mesenchymal cells expressing heterogeneous levels of VGCCs and CRAC channels, thereby allowing synchronized Ca2+ oscillations to occur and coordinate directional cell movements.


Electric currents and ion channel expression in feathers

A vibrating probe11 was used to measure endogenous DC electric currents on intact chicken embryos from Hamburger & Hamilton18 (H&H) stage 29–38 (Fig. 1a). Measurement locations included interbud regions (between feather buds), anterior and posterior feather bud regions. Inward currents were observed in interbud regions for all developmental stages examined. Inward ionic currents were also observed in feather buds before the initiation of polarized elongation (H&H 29–34). Following the onset of elongation (H&H 34–35), the current direction at the anterior bud regions reversed, while current directionality remained inward at posterior bud regions. We hypothesize that these dynamic changes of endogenous feather bud ionic currents result from spatiotemporally regulated ion channel expression and activity.

Fig. 1
figure 1

Dynamic bioelectric currents and expression of Ca2+-related channels in elongating feathers. a Endogenous electric current density in anterior, posterior feather buds and interbud regions in intact chicken embryos at different developmental stages (n = 9–11 measurements per position per stage). Between Hamburger & Hamilton (H&H) Stage 34–35, the direction of currents at the anterior buds reversed from inward to outward, while that at the posterior buds stayed inward. The direction of currents at interbud regions stayed inward throughout the developmental stages examined. Data are presented as mean ± s.e.m. **P < 0.005 (two-sample Student’s t test). Scale bar, 500 μm. b Confocal image of H&H 31 and H&H 35 feather buds stained with LCAM and VIM to reveal distinct morphology of epithelial and mesenchymal cells. VIM positive cells in epithelium are melanocytes and periderm cells. Dashed lines highlight epithelial-mesenchymal boundaries. Scale bars, 50 μm. c Screening of genes encoding ion channels in RNA-Seq highlights multiple Ca2+-conducting channels. d In situ hybridization results of genes encoding components of VGCCs, gap junctions, CRAC channels, and Ca2+-activated K+ channels. Scale bar, 50 μm

To screen candidates for the ion channels involved in stage-dependent current changes, we compared the transcriptomes of H&H 31 and H&H 35 embryonic chicken dorsal skins (Supplementary Fig. 1), with epithelium and mesenchyme separated due to their distinct cell morphology and molecular expression (Fig. 1b). Epithelium is primarily comprised of cuboidal cells tightly arranged in a honeycomb pattern (highlighted by staining of LCAM, Liver Cell Adhesion Molecule), while mesenchyme is mainly composed of VIM (Vimentin) positive, bipolar, or multipolar fibroblasts (Supplementary Fig. 2a, b). Neurites are very rare and only exist in mesenchyme underneath feather buds during feather elongation (Supplementary Fig. 2c). We focus on Ca2+ channel coding genes in RNA-Seq analysis, because Ca2+ ions not only serve as carriers of inward currents19, but also second messengers to link membrane potentials to downstream cellular events20. Intercellular gap junction channels were also included, as they are crucial to establish tissue-wide electrical paths21. Ca2+-activated K+ channels carrying outward currents may help restore the resting membrane potential after depolarization-induced Ca2+ influx22.

To shorten the candidate gene list (Supplementary Data 1), the following filter condition was applied: minimum RPKM (reads per kilobase of transcript per million mapped reads) > 1.5, fold change > 1.3 (before Log2 transformation), P < 0.05 (Fig. 1c). Afterwards, RNA in situ hybridization and RT-qPCR were performed to validate the RNA-Seq results (Fig. 1d and Supplementary Fig. 3). L-type and T-type voltage-gated Ca2+ channels (VGCCs), gap junctions and Ca2+ release activated Ca2+ (CRAC) channels exhibited developmental stage-dependent variations of expression. Connexin-43 gap junctions were localized at the posterior–distal epithelium and mesenchyme until feather elongation when the expression region expanded in the mesenchyme. Meanwhile their expression level decreased in the epithelium. STIM1 (Stromal Interaction Molecule 1, Ca2+ sensor of CRAC channels) was expressed with a similar pattern as Connexin-43 in feather mesenchyme. The binding partner of STIM1 (ORAI1, ion conducting pore subunit of CRAC channels) was also present in feathers but exhibited no stage-dependent variation in expression. Furthermore, in situ hybridization detected sparse KCNMA1 (component of Ca2+-activated K+ channel) expression in anterior epithelium and basal mesenchyme of H&H 35 feather buds.

Functional VGCCs and Connexin-43 gap junctions in feathers

To visualize cytoplasmic Ca2+ buildup due to influx through functional VGCCs in feathers, we constructed an avian viral vector (RCAS) expressing Ca2+ sensor GCaMP6s10, T2A peptide, and mCherry. By normalizing the fluorescence intensity of GCaMP6s to that of mCherry, changes in Ca2+ levels could be measured and compared among tissues despite heterogeneous levels of viral expression. To visualize cytosolic Ca2+ changes along both the transverse and sagittal planes, we adopted skin explants and strip configurations (Fig. 2a). As expected, KCl application to depolarize membrane potentials triggered Ca2+ increases in mesenchymal but not epithelial cells. The responses elevated as the feathers developed (Fig. 2b–f, k; Supplementary Fig. 4a; Supplementary Movies 15). Pretreating skins with a VGCC blocker, Nifedipine, dramatically reduced the KCl response (Fig. 2g, k and Supplementary Movie 6). To measure direct currents through VGCCs, H&H 35 mesenchyme was dissociated to single cells for patch clamp experiments (Supplementary Fig. 5). Consistent with the in situ hybridization data (Supplementary Fig. 3a), a current–voltage (I–V) plot supports the presence of functional VGCCs. The measured I–V curve indicates that the cells mainly expressed T-type VGCCs, but we cannot exclude the possibility that a cell population may express L-type VGCCs due to the limited number of tested cells used in the patch clamp experiment. KCl-induced fast Ca2+ increases were also observed in cultured single cells (Fig. 3a, b ROI 1 and Supplementary Movie 7). Taken together, our data suggest that active VGCCs are present in a subpopulation of feather mesenchymal cells.

Fig. 2
figure 2

Functional VGCCs, gap junctions and CRAC channels in elongating feathers. a Schematic drawing exhibiting the skin explant and strip configuration used for time-lapse Ca2+ imaging. Bright field images of feather buds at different developmental stages in skin explants and strips are shown. Dotted lines highlight epithelial-mesenchymal boundaries. Scale bars, 50 μm. bd Time-lapse Ca2+ imaging of feathers from skin strips at different stages (n = 3 for each stage). Dotted lines indicate regions of interest (ROI) for quantification (′′ denotes seconds). Pseudocolor images of the ratios are presented at selected time points (arrowheads). Scale bar, 50 μm. e Quantifying change of mesenchymal Ca2+ increases in feathers from skin strips. Ro: baseline F GCaMP6s/F mCherry ratio before KCl application. ΔR: the peak ratio subtracts Ro. Mean ± s.e.m. *P < 0.05 (Wilcoxon rank test). Dots represent individual data points. f Time-lapse Ca2+ imaging of feathers in skin explants at H&H 35 (n = 16/16). g Pretreatment with 50 μM Nifedipine for 3 min greatly dampened the KCl-induced Ca2+ elevation (n = 4/4). h Pretreatment with 150 µM Carbenoxolone for 30 min significantly reduced the KCl response (n = 4/4). i Feather buds pretreated for 30 min with 0 mM Ca2+ solution including 10 µM Thapsigargin exhibited notable Ca2+ influx after perfusion of 2 mM Ca2+ solution (n = 3/3). j 5 µM BTP2 significantly reduced the Ca2+ influx (n = 3/3). k Quantification of Ca2+ response in feathers from skin explants under different treatments. Mean ± s.e.m. *P < 0.05 (Wilcoxon rank test)

Fig. 3
figure 3

Heterogeneous Ca2+ responses in cultured mesenchymal cells. a, b Three types of Ca2+ responses upon 100 mM KCl stimuli in H&H 35 single mesenchymal cells: KCl-induced Ca2+ increase (ROI 1, n = 24/73), biphasic Ca2+ response (ROI 2, n = 7/73), KCl-induced Ca2+ decrease (ROI 3, n = 42/73). Rectangles denote regions of interest (ROI) for quantification. AM-Fura-2 dyes were used to measure Ca2+ level by excitation wavelength of 350 nm (F350) and F380. Scale bar, 25 μm. ′ denotes minutes. Whisker bottom, box bottom, median line, box top, and whisker top correspond to 10, 25, 50, 75, and 90 percentile.  c, d 10 μM Nitrendipine (Nitren) or 10 μM LaCl3 was used to inhibit L-type VGCC (n = 5) and CRAC channels (n = 20), respectively. **P< 0.01 (Wilcoxon rank test). e Mesenchymal cells were identified by vimentin staining after Ca2+ measurements. Scale bars, 35 μm, 110 μm. f Fast application of KCl solution for 10 s induced immediate Ca2+ responses. Four cells labeled with colored numbers in e were chosen to plot the ratios. ′′ denotes seconds. g Slow, gentle bath perfusion of KCl (indicated by the time delay between onset of KCl application and response) implies the response is not an artifact of shear stress stimulation. h Negative correlation between Ro and KCl-induced Ca2+ increase (Red circle, fast application/bath perfusion, n = 246). Positive correlation between Ro and KCl-induced Ca2+ decrease (Black circle, fast application, n = 184; blue circle, bath perfusion, n = 62). % increase or decrease of Ca2+ response was calculated by ∆R/Ro

To confirm the presence of functional gap junction channels, we performed the scrape-loading/dye transfer assay to confirm the permeability of gap junctions in feathers23. In H&H 35 feather buds Lucifer yellow quickly spread to almost all feather mesenchymal cells after scraping (Supplementary Fig. 6a, b). Pretreatment of the skin for 1 h with 18-α-GA, which disrupts the Connexin-43 arrangement within the channel24, dramatically reduced intercellular transfer of Lucifer yellow (Supplementary Fig. 6a). Similar results were observed in samples treated with PMA (Supplementary Fig. 6b), which activates PKC to alter Connexin-43 phosphorylation and downregulates Connexin-43 expression25,26,27,28. As gap junction communication plays a role in propagating electrical signals among cell populations29, we expected weaker KCl responses in feathers after administering gap junction blockers. Indeed, pretreating the skins with either Carbenoxolone (an 18-α-GA derivative) or PMA significantly reduced the KCl responses (P < 0.05, Wilcoxon rank test, Fig. 2h, k, Supplementary Fig. 6c and Supplementary Movies 8, 9). These data indicate that a functional gap junction network exists in feather mesenchyme.

Functional CRAC channels in elongating feathers

CRAC channels are activated by depleting the endoplasmic reticulum (ER) Ca2+ stores. To assess CRAC channel expression in feathers, intact skin explants were bathed in EGTA-buffered Ca2+ free solution containing Thapsigargin (ER Ca2+ pump blocker). After Thapsigargin treatment, 2 mM Ca2+ Ringer’s solution was applied to induce store-operated Ca2+ influx. Notable Ca2+ influx was observed in both feather epithelium and mesenchyme (Fig. 2i, k and Supplementary Movie 10). The CRAC channel inhibitor, BTP230, dramatically reduced Ca2+ influx (Fig. 2j, k and Supplementary Movie 11). Taken together, feather buds express functional CRAC channels.

In dissociated single mesenchymal cells, uncoordinated, spontaneous, and long-lasting Ca2+ fluctuations were observed (Fig. 3a ROI 2, 3). Normally, high KCl stimulation causes a rapid rise in Ca2+, owing to membrane depolarization leading to opening of VGCCs. This was, indeed, observed in many cells (Fig. 3a, b ROI 1). Surprisingly, KCl-induced Ca2+ decreases were also observed in some cultured mesenchymal cells (Fig. 3a, b ROI 3). We hypothesize that the decrease might be due to membrane depolarization shutting off Ca2+ influx through the inwardly rectifying CRAC channels31. Some cells exhibited biphasic responses to KCl (a rapid rise, followed by a decrease), possibly due to the cells’ expressing both VGCCs and CRAC channels (Fig. 3a, b ROI 2). When KCl was applied along with Nitrendipine, a VGCC blocker, Ca2+ levels showed only the decrease, confirming the role of VGCCs in the rapid upward spike in the biphasic response (P < 0.01, Wilcoxon rank test, Fig. 3c, d). The KCl-induced decrease, even with Nitrendipine, suggests that the cells may express constantly active CRAC channels in addition to VGCCs (Fig. 3c and Supplementary Movie 12). Application of lanthanum (La3+), a CRAC channel pore blocker, significantly decreased the baseline cytoplasmic Ca2+ levels in some cells, which also indicates the presence of sustained active CRAC channel currents (P < 0.01, Wilcoxon rank test, Fig. 3c, d and Supplementary Movie 13). Additionally, heterogeneous responses to Ca2+ stimulation after Ca2+ deprivation were observed in the dissociated mesenchymal cells, confirming the non-uniform presence of CRAC channels (Supplementary Fig. 7a-d). Finally, biphasic KCl responses were also observed in feather bud mesenchyme under skin strip configuration (Supplementary Fig. 8a, b and Supplementary Movie 14), implying the presence of active CRAC channels in vivo.

While we tried to classify the subpopulations of the mesenchymal cells with respect to KCl-induced Ca2+ responses, we discovered that there was a correlation between cell morphology and Ca2+ responses. Surface area and aspect ratio measured in VIM staining images indicated that smaller- and/or thin-shaped cells tended to exhibit elevated baseline Ca2+ levels and KCl-induced Ca2+ decreases, while larger- and/or polygonal-shaped cells tended to exhibit KCl-induced Ca2+ increases (Fig. 3e–h and Supplementary Fig. 7e, f). The elevation of baseline Ca2+ could be abolished by Thapsigargin treatment, implying contributions from constantly active CRAC channels (R0 of Fura-2 is about 0.5 in all cells measured in Supplementary Fig. 7a, b) Notably, some mesenchymal cells located at the anterior region of buds were elongated compared to ones located at the posterior region (Supplementary Fig. 2a, b). Therefore, we speculated that subpopulations of dissociated mesenchymal cells somehow retain their endogenous locational information which causes them to express the functional Ca2+ channels corresponding to their sites of origin.

To further evaluate the contribution of CRAC channels to the dynamic Ca2+ changes in feather buds, we created light-activated CRAC channels called opto-cCRAC by fusing the chicken cytosolic STIM1 domain with the LOV domain from Avena sativa phototropin 132. STIM1 is located in the ER membrane, where normally, upon depletion of the ER, it activates the plasma membrane ORAI channels. Upon blue light illumination, the LOV domain undergoes conformational changes, exposing the STIM1 cytosolic domain to engage ORAI channels on the cell membrane. We confirmed that the opto-cCRAC can induce Ca2+ influx in Hela cells (Fig. 4a and Supplementary Movie 15) and H&H 35 mesenchymal cells (Fig. 4b and Supplementary Movie 16). When we artificially elicited Ca2+ oscillations by cyclic activation of opto-cCRAC in skin explants transduced with RCAS virus encoding opto-cCRAC for 48 h, the highly infected feathers were significantly elongated compared to the poorly infected ones on the contralateral side (P < 0.01, Wilcoxon rank test, Fig. 4c). Control skins transduced with RCAS virus encoding GCaMP6s-T2A-mCherry exhibited no discernible feather morphology changes. Thus collective cell Ca2+ oscillations are crucial for feather elongation.

Fig. 4
figure 4

Ca2+ influx induced by cyclic activation of opto-cCRAC enhances feather elongation. a In Hela cells opt-cCRAC induced Ca2+ influx after blue light exposure (n = 20/20). jRCaMP1b was expressed to detect Ca2+ level changes. Arrowheads in the line plot highlight the time point of images on the left. F/F0, changes in fluorescence. Mean ± s.d. Scale bar, 10 µm. b Light-induced Ca2+ influx occurred in H&H 35 mesenchymal cells infected by virus encoding opto-cCRAC (cyan rectangles, n = 25/43) but not in the uninfected cells (magenta rectangles, n = 0/33). Mean ± s.d. Scale bar, 10 µm. (′′ denotes seconds). FE: fluorescence at the end of recording (70′′); **P < 0.01 (Chi-square test). c After 48 h cyclic blue light illumination, skin regions (n = 8/10) highly expressing opto-cCRAC developed more elongated feathers than the poorly infected buds (n = 60 for each group, **P < 0.01, Wilcoxon rank test). No discernable feather morphology changes (n = 48, NS, not significant, Wilcoxon rank test) were observed in skins infected by RCAS-GCaMP6s-T2A-mCherry. Regions close to the dorsal mid-line were magnified (rectangles) to compare feather aspect ratio (ellipses). Scale bar, 500 µm. Customized boxplot: Mean (red) ± s.d. (pink), 95% confidence interval (violet). Dots denote individual data points

Ca2+ oscillation patterns modulate feather elongation

To directly visualize the dynamics of the tissue Ca2+ profile, we did 4D (3D space + time) imaging of elongating feathers from H&H 34 skin explants and strips infected with RCAS virus encoding GCaMP6s-T2A-mCherry. Intriguingly, not only did we see fast, sporadic Ca2+ transients on the scale of seconds (Supplementary Fig. 8c, e and Supplementary Movie 17), we also observed slow Ca2+ oscillations, which are generally synchronized (peaks and valleys in phase) in anterior and posterior mesenchyme (Fig. 5a, Supplementary Fig. 8d, e and Supplementary Movies 1821). The oscillating zone slowly expands in the anterior–proximal direction at about 1.7 μm/min (Fig. 5a and Supplementary Fig. 8d, f). These oscillations are dramatically dampened upon the inhibition of VGCCs or gap junctions, although some sparse Ca2+ transients could still be spotted (Fig. 5a; Supplementary Fig. 6d and Supplementary Movies 2227). Thus VGCCs and gap junction channels are required for multicellular Ca2+ oscillations during feather elongation.

Fig. 5
figure 5

Modulating physiological Ca2+ oscillations alters feather elongation process. a Virtual sections of 4D ratiometric Ca2+ imaging of elongating feather buds on H&H 34 skins (n = 3). ROI analysis of GCaMP6s and mCherry fluorescence ratio exhibited synchronized Ca2+ oscillations in anterior (cyan rectangle) and posterior (magenta rectangle) mesenchyme. The high Ca2+ area expanded anteriorly over time (the intersection of cyan and magenta lines).′ in x-axis denotes minutes. Pseudocolor ratiometric images were shown at selected times (arrowheads). 50 μM Nifedipine or 150 μM Carbenoxolone treatment dramatically reduced the number of cells showing elevated Ca2+ (n = 2). Scale bar, 50 μm. b Feather buds on H&H 31 skins became elongated filaments oriented posteriorly after 4-day culture with DMSO (red arrows, n = 10/10). Nifedipine-treated feather buds were shorter and had no apparent anterior–posterior polarity (n = 8/8). 150 μM Carbenoxolone treatment inhibited feather elongation and disrupted feather polarities (red arrows, n = 6/6). H&E: Hematoxylin and Eosin staining. Scale bars, 500 μm (whole-mount skin), 50 μm (section). c In H&H 35 Skins, the regions (n = 4/4) infected with lentivirus encoding Connexin-43 shRNA (pLL3.7-Cx43-SH) exhibited dramatically inhibited elongation of young feather buds (cyan ellipses) compared to the control side (magenta ellipses, n = 23 for each group, **P < 0.01, Wilcoxon rank test). Rectangles highlight magnified area. Scale bar, 500 µm. Customized boxplot: Mean (red) ± s.d. (pink), 95% confidence interval (violet). Dots denote individual data points

Next we explored whether the alterations of physiological Ca2+ dynamics would change feather morphology. We treated the skin with Nifedipine, Carbenoxolone, PMA, and another gap junction inhibitor Mefloquine33 for 4 days and compared feather morphology to the untreated controls (Fig. 5b and Supplementary Fig. 9). The control feathers developed into elongated filaments tilting posteriorly. Nifedipine-treated feathers grew upward for a while and then stopped, without developing an apparent anterior–posterior (A–P) polarity. Carbenoxolone and Mefloquine-treated feathers were also shorter than the controls. PMA treatment induced more severe phenotypes than Carbenoxolone in that feather buds disappeared in some skin regions. This difference may result from downstream effects of PKC signaling other than gap junction inhibition. We also genetically perturbed gap junction expression levels using lentivirus encoding Connexin-43 shRNA (pLL3.7-Cx43-SH)34. The infected feather buds were notably shorter than the counterparts in the contralateral, virus-negative side (P < 0.01, Wilcoxon rank test, Fig. 5c). All the chemicals also significantly altered the feather aspect ratio (P < 0.01, Wilcoxon rank test), while none of them significantly increased cell apoptosis (Supplementary Fig. 9). Nifedipine treatment increased cell proliferation while Mefloquine treatment had the opposite effect. Taken together, neither cell proliferation nor apoptosis is a major process involved in oriented feather elongation.

VGCCs and gap junctions modulate mesenchymal cell migration

Since feather elongation is mainly driven by cell rearrangement during development16, we scrutinized cell movement patterns by tracking individual mesenchymal cells labeled with histone-H2B GFP in skin explants. Since there was a strong correlation between Ca2+ dynamics and feather morphology changes as shown above, we tested the effect of VGCC and Gap junction blockers on cell migration. We segmented out the feather mesenchyme to exclude epithelial cells, tracked cell positions over time, and plotted trajectories along the X (anterior–posterior), Y (left–right), and Z (proximal–distal) axes (Fig. 6a). We also quantified the mean cell movement velocity by averaging every cell’s displacement over time (Fig. 6b), as well as cell movement directions (displacement angle) in the XZ plane by calculating the inverse tangent of their displacement along the Z and X axes (Fig. 6c). In control skins, the feather mesenchymal cells move upward and posteriorly in a pulsatile manner, meaning there are moments when the migration halts (Fig. 6 and Supplementary Movie 28). When we compare mesenchymal cell migration patterns in the anterior and posterior bud regions, those in the anterior half move slower than their posterior counterparts, consistent with previous cell tracking data16, but their movement directions are similar (Supplementary Table 1 and Supplementary Fig. 10a). In Nifedipine-treated skins, feather mesenchymal cells mainly moved upward without notable A–P bias (Supplementary Movie 29). The movement velocity and displacement angle are similar between the anterior and posterior bud mesenchymal cells (Supplementary Table 1 and Supplementary Fig. 10b). Carbenoxolone treatment also diminished cell movement in the posterior direction (Fig. 6c and Supplementary Movie 30). In PMA-treated skins, feather mesenchymal cells mainly move downward and anteriorly (Supplementary Fig. 10c and Supplementary Movie 31), which explains why some feather buds disappeared in long-term culture (Supplementary Fig. 9a). Therefore, blocking VGCCs and gap junctions dramatically altered the mesenchymal cell movement patterns, especially the directionality.

Fig. 6
figure 6

Altered feather mesenchymal cell migratory patterns upon inhibition of VGCCs and gap junctions. a 4D cell nucleus (H2B-GFP) imaging of elongating feather buds on H&H 34 skins. Left-most panel, 3D rendering of the feather buds at Time 0, with the mesenchyme highlighted in white. Middle panel, Mesenchymal cell nuclei were segmented (green dots) and their displacement vectors (yellow arrows) were mapped. Right panel, Cell movement trajectories. Different trajectory colors represent time (′ denotes minutes). Scale bar, 50 μm. b Plotting individual mesenchymal cell positions along the X (anterior–posterior), Y (left–right), and Z axis (up–down) over time. Black line indicates averaged cell position over time. The averaged velocities ( is the averaged displacement along the corresponding axis divided by time) are shown above each plot. c Angle histogram plots illustrate the cell displacement angle in the XZ plane (0°, 90°, 180°, and 270° represent posterior, upward, anterior, and downward directions, respectively). Cells tracked: n = 378 for controls, n = 316 for Nifedipine, and n = 278 for PMA-treated samples. The averaged displacement angles (ϴ̅) were significantly altered upon Nifedipine or PMA treatment. **P< 0.01 (Watson’s U2 test)

SHH signaling allows sporadic Ca2+ transients to synchronize

Next, we explored the biochemical signals that modulate Ca2+ oscillation and cell migration patterns. The Ca2+ oscillations in elongating feathers initially emanate from the posterior–distal mesenchyme, which is known as the SHH signal responding zone. SHH is expressed in the posterior–distal epithelium while its receptor PTCH1 is enriched in the underlying mesenchyme (Fig. 7a). Therefore, SHH protein from the feather epithelium must have diffused through the basement membrane into the mesenchyme. To confirm SHH signaling activity in the posterior–distal mesenchyme, we infected embryonic chicken skin with a virus-based reporter construct, RCAN-GBS-GFP35. The GLI-binding-site (GBS) drives gene expression upon SHH signal activation, while RCAN itself has no internal promoter activity. We found that GFP-positive cells co-localize with the PTCH1-positive region (Fig. 7a). The GFP-positive zone expanded in the anterior–proximal direction as feathers elongated, resembling the expansion pattern of synchronized Ca2+ oscillations. Furthermore, blocking SHH signaling with Cyclopamine36 causes failure of feather bud polarization and elongation (Fig. 7b). This morphological abnormality could be fully rescued by adding the SHH agonist SAG36 (Supplementary Fig. 9), and partially rescued by opto-cCRAC together with cyclic blue light illumination. The feather mesenchymal region enriched for opto-cCRAC elongated and became the new feather tips (Fig. 7c). In 4D Ca2+ imaging, Cyclopamine treatment inhibited synchronized Ca2+ oscillations, but sporadic Ca2+ transients were still observed (Fig. 7d and Supplementary Movies 3234). When we track mesenchymal cells in Cyclopamine-treated feathers, they initially move upward, then stop and move slightly downward (Fig. 7e, f and Supplementary Movie 35). The anterior and posterior mesenchymal cell populations have significant differences in movement directionality: the anterior cells move more anteriorly while the posterior cells mainly move upward (P < 0.01, Watson’s U2 test, Supplementary Fig. 10d).

Fig. 7
figure 7

SHH signaling underlies normal Ca2+ oscillation and mesenchymal cell migration pattern in feather. a In situ hybridization reveals that SHH is expressed in the posterior–distal epithelium while PTCH1 is enriched in the underlying mesenchyme. An RCAN virus-based GLI reporter demonstrates expansion of the mesenchymal SHH-responding zone anteriorly during feather elongation. Scale bar, 50 μm. b H&H 31 skins cultured for 4 days in 5 μM Cyclopamine exhibited dramatic inhibition of feather bud elongation (ellipse, n = 8/8). Scale bars, 500 μm, 50 μm. c Expression of opto-cCRAC in feather mesenchyme and cyclic blue light illumination partially rescued the Cyclopamine mediated inhibition of elongation by inducing new feather tips to form (n = 3/3). The buds with new tips exhibited more elongated morphology (cyan ellipse) than those poorly or not infected ones (magenta ellipse, n = 29 for each group, **P < 0.01, Wilcoxon rank test). Rectangles highlight magnified area. Scale bars, 500 μm. Customized boxplot: Mean (red) ± s.d. (pink), 95% confidence interval (violet). Dots denote individual data points. d Virtual sections of 4D Ca2+ imaging of H&H 34 feather buds treated with 5 μM Cyclopamine (n = 2). Scattered Ca2+ fluctuations were observed among the cells. Quantification of F GCaMP6s/F mCherry was conducted for the anterior (cyan rectangle) and posterior (magenta rectangle) mesenchyme and demonstrated in line plot. Scale bar, 50 μm. e 9 h 4D cell nuclear imaging of a feather bud treated with 5 μM Cyclopamine (mesenchyme highlighted in white). Scale bar, 50 μm. f Mesenchymal cell positions plotted over time and the averaged displacement angles (n = 430)

SHH/WNT signaling module activates Connexin-43 expression

Disruption of Ca2+ oscillation patterns upon Cyclopamine treatment implies a role of SHH signaling in regulating either the activities or expression levels of certain Ca2+-related channels. Previous studies of Xenopus spinal cells implicated SHH signaling in increasing spontaneous neuronal Ca2+ transients36. We conducted similar experiments in cultured H&H 34 mesenchymal cells but observed no significant increase of spontaneous Ca2+ transients upon treatment with SHH N-terminus protein or SAG compared to the controls (Wilcoxon rank test, Supplementary Fig. 11a and Supplementary Movie 36). We also examined KCl response strength in feathers with short-term Cyclopamine (Supplementary Movie 37) or SAG (Supplementary Movie 38) treatment, but no notable changes were observed, either (Supplementary Figs. 4 and 11b). Therefore, we assume that SHH signaling mainly affects channel gene expression, which takes longer to occur. We attempted to identify SHH-induced Ca2+ channel genes in an embryonic context through RCAS mediated SHH overexpression. However, this led to severe developmental defects before feather buds emerge (Supplementary Fig. 12a). Hence, we switched to cultured mesenchymal cells for the answer. qPCR results indicate 24-hr SHH N-terminus protein treatment mildly elevated Connexin-43 and STIM1, but not CACNA1C or PKD2 expression (Fig. 8a and Supplementary Fig. 12b). In skin explants, 48-hr SAG treatment also elevated Connexin-43 expression in feathers, while Cyclopamine treatment had the opposite effect (Fig. 8b). The mild effect of SHH protein on Connexin-43 expression in cultured mesenchymal cells may implicate the involvement of other epithelial factors in inducing Connexin-43 expression, as epithelium is absent in the cell culture. Previously we discovered active WNT/β-catenin signaling in posterior feather mesenchyme16. During feather elongation, the WNT-responding zone (composed of nuclear β-Catenin positive cells) expands distally and partially overlaps with the SHH-responding zone (Fig. 8c). Therefore, we examined how WNT signaling regulates Connexin-43 expression. RCAS enforced expression of constitutively active β-Catenin in chicken embryos substantially upregulated Connexin-43 expression (Fig. 8d). Meanwhile no elevation was observed in control (RCAS-GCaMP6s-T2A-mCherry) embryos (Supplementary Fig. 12a). The RCAS-β-Catenin infected feather buds also exhibited randomized polarity as seen previously16. In skin explants treated with LiCl, which activates WNT/β-catenin signaling37, we also observed elevated Connexin-43 expression (Supplementary Fig. 12c), while the inhibition of WNT/β-catenin signaling by endo-IWR138 had the opposite effect (Supplementary Fig. 12c). qPCR of cultured mesenchymal cells also demonstrated an elevation of Connexin-43 expression upon LiCl treatment, which is enhanced by SHH N-terminus protein treatment (Fig. 8a). Additionally, we searched for the SHH-responding motif (GLI-binding site) and WNT-responding motif (LEF1-binding site) in the active Connexin-43 promoter region, which is marked by enrichment of Histone H3 Lysine 4 trimethylation39 in ChIP-Seq analysis. We pinpointed a GLI-binding site and a LEF1-binding site in proximity (Fig. 8e), supporting the idea that SHH and WNT signaling may work together to activate Connexin-43 transcription. Such a synergistic effect was not seen for CACNA1C, STIM1, or PKD2 expression (Supplementary Fig. 12b).

Fig. 8
figure 8

SHH and WNT signaling synergistically activate Connexin-43 expression. a qPCR revealed a mild elevation of Connexin-43 expression in cultured mesenchymal cells treated for 24 h with 0.25 µM SHH N-terminal peptide (N-SHH) or 7 mM LiCl to activate WNT signaling. The upregulation is more significant when both N-SHH and LiCl are present. Activation of SHH and WNT signaling are confirmed by PTCH1 and LEF1 qPCR, respectively (n = 6). **P < 0.01, two-sample Student’s t test. Customized boxplot: Mean (red) ± s.d. (pink), 95% confidence interval (violet). Dots denote individual data points. b In situ hybridization demonstrated higher Connexin-43 expression in feather buds treated with 500 nM SAG for 48 h. 5 μM Cyclopamine treatment decreased Connexin-43 expression. Scale bar, 50 μm. c Immunostaining revealed close proximity of the Connexin-43 positive zone and nuclear β-Catenin zone in feather mesenchyme. Scale bar, 50 μm. d Mis-expressing constitutively active β-Catenin induced site-specific elevation of Connexin-43 expression and abnormal feather polarity (n = 5/5). The region magnified is highlighted by rectangle. Scale bar, 500 µm. e Motif search in the active promoter region (Histone H3 Lysine 4 trimethylation, blue bar) of Connexin-43 identifies LEF1 and GLI-binding sites in close proximity. Orange peaks highlight enrichment levels


Emergence of organized patterns from apparently random cells is the essence of tissue morphogenesis40. During tissue morphogenesis, cells navigate through a three-dimensional space to interact and organize themselves into proper configurations. Using time-lapse imaging and tracking, we observed dynamic and multi-dimensional cellular flows in the 4D context. Random and directed movements seem to co-exist in mesenchymal subpopulations. Cellular collectives form, disassemble, then reform. Cells move in one direction, stop, and then reorient. Amazingly, order gradually emerges from these seemingly chaotic movements, and organs with proper shape and orientation emerge. It is difficult to explain such complex choreography just with chemotaxis. The roles of mechanical force, bioelectric signals and ionic control in morphogenesis are now gaining increasing attention41,42. Here we leverage the distinct feather patterns on developing chicken skins to explore the correlation between biochemical cues, bioelectric signals and Ca2+ dynamics in collective cell behavior control.

Before the onset of feather buds elongation, the EF around chicken dorsal skin is relatively homogenous and inwardly directed. Outward currents likely exist in other regions of the chicken embryo to complete the circuit on a global scale, which is known to occur in earlier chicken embryos43. These global circuits have also been detected in zebrafish embryos and Xenopus tadpoles11,44. Later on the current direction reverses locally at the anterior side of feather buds in chicken embryos. Another case of local electric current reversal is reported before limb bud formation in the Xenopus embryos45. Thus local circuit formation may signify and participate in orchestration of local collective cell behaviors in different biological processes.

We postulate that the formation of these local electric circuits during feather bud elongation relies on active VGCC, CRAC, Ca2+-activated K+ channels, as well as the gap junction network. Previously, gap junction components have been detected in multiple types of skin appendages including feathers46,47,48 and their networks are known to shape multicellular Ca2+ activities in a variety of excitable and non-excitable cells49. Due to their permeability to ions and small molecules, gap junctions serve as low-resistance pathways to spread ionic currents, and hence propagate membrane potential changes among neighboring cells21,29. The range of the gap junction network is regulated by diffusible morphogens from the biochemical signaling centers, including SHH diffused from distal placode epithelium50 and WNT7A diffused from posterior bud epithelium15. Since both morphogens are capable of inducing Connexin-43 expression, their overlapped area will be electrically coupled to the best degree. This is consistent with the fact that the Ca2+ oscillations start at posterior–distal mesenchyme and gradually expand in area along the anterior–proximal direction. Meanwhile the expansion speed is slower than Ca2+ wave propagation speeds reported in most other systems51, implying Ca2+ diffusion is not the rate-limiting step of this process. Additionally, in situ hybridization and in vitro qPCR data (Fig. 1c and Supplementary Fig. 12b) imply that SHH and WNT signaling likely also upregulate STIM1 expression, which enables store-operated Ca2+ influx through CRAC channels. In dissociated H&H 35 feather mesenchyme, we observed sparse cells with changes in cytosolic Ca2+. Those cells that did show Ca2+ changes typically exhibited sustained Ca2+ elevations, implying continuous CRAC channel activation. Though sustained CRAC activity may depolarize membrane potential to activate the low-threshold voltage-gated T-type Ca2+ channels, tissue-wide synchronized Ca2+ oscillations were not observed until gap junction expression increased in mesenchyme. Thus we think gap junction mediated electric coupling is essential for synchronizing the originally heterogeneous VGCC and CRAC activation events, transforming sporadic Ca2+ transients into organized oscillations. These oscillations facilitate the collective cell movements mediating feather elongation in the posterior–distal direction (Fig. 9).

Fig. 9
figure 9

Biochemical and bioelectric signals guiding directed mesenchyme cell migration in feather. SHH and WNT7A protein produced in the epithelium diffuse into the underlying mesenchyme to induce the SHH and WNT-responding zone, respectively. Together they activate Connexin-43 expression to compose intercellular gap junction channels. Heterogeneously distributed VGCCs and CRAC channels contributed to the inward current observed at posterior–distal part of elongating feathers, while activation of Ca2+ -activated K+ channels may contribute to the outward current at anterior-basal part of feathers. The gap junction network establishes a low-resistance electrical path across feather mesenchyme, homogenizing differential Ca2+ channel activities among cells to allow synchronized Ca2+ oscillations to form. These slow oscillations coordinate the collective migration of mesenchymal cells. Meanwhile much faster Ca2+ transients occur sporadically in individual cells

Ca2+ fluctuations have previously been implicated in modulating cell migration52,53,54, convergent extension51, apical constriction55, etc. Our study demonstrates slow multicellular Ca2+ oscillations coordinate collective mesenchymal cell migration in skin appendage organogenesis. We have three hypotheses of how these two events are linked: (1) Elevated cytoplasmic Ca2+ promotes myosin-driven cell protrusions by activating myosin light chain kinase (promoting actomyosin contractility)51. (2) Elevated mitochondrial Ca2+ (mitochondria are known to at least partially buffer cytoplasmic Ca2+ increase) enhances ATP production56. (3) The oscillations serve as a communication mechanism enhancing sensitivity to gradients of chemotactic cues like FGF57,58,59,60. Since FGF signaling is required for normal SHH expression in feather60, the chemotaxis and gap-junction-based communications may function in parallel.

Multicellular Ca2+ oscillations are dependent on both gap junctions and CRAC channels in cells lacking VGCCs61. Our in situ hybridization data indicates that the Connexin-43 expression region overlapped with that of STIM1 in feather mesenchyme. Although CRAC channel inhibitor BTP2 did not block feather elongation (Supplementary Fig. 9), oscillatory activation of opto-cCRAC channels did enhance feather elongation (Fig. 4c). Beside VGCCs and CRAC channels, Ca2+ transients could also be triggered by stretch-activated Ca2+ channels62, interestingly, the stretch-activated Ca2+ transients observed in human gingival fibroblasts are also contributed by VGCCs, suggesting a potential link between the two types of channels. Furthermore, mechanical stimulations could regulate the expression, subcellular localization and even phosphorylation state of Connexin-4363. There is a possibility that stretch between cells during feather mesenchymal migration helps reshape the functional gap junction network.

The mechanism described in this work is active when feather primordia ( < 100 μm in length) elongate to become long feather buds ( > 200 μm in length), representing a substantial change in the organ aspect ratio. Unlike the more stable adhesion molecule-mediated cell condensates, this mechanism enables transient cell collectives to form dynamically, effectively guiding mesenchymal cells during the construction of organ architectures. This study also demonstrates a proof-of-concept that manipulation of Ca2+ patterns can modulate cell behaviors in tissues and organs located close to the body surface. Hence, the optogenetic Ca2+ channels would have wide applications in procedures such as accelerating wound healing, decreasing scar formation, wound contraction, and inducing hair regeneration.


Egg resources

Animal care and experiments were conducted according to the guidelines established by the USC Institutional Animal Care and Use Committee. White leghorn chicken eggs were purchased from Charles River (pathogen free) and AA laboratory.

Vibrating probe measurement of feather bioelectric currents

The vibrating probe technique for non-invasive measurement of endogenous electric current densities has been previously described11. The probe is an Elgiloy-stainless microelectrode (WPI #SSM33A70) coated with a thin layer of parylene insulation, leaving 1–2 µm of metal exposed at the tip. Using a nano-amp power supply, we electroplate a thin layer of gold and then a platinum ball onto the tip. The probe, mounted on a 3-dimensional micro-positioner (Line Tool Co., model H), is vibrated at high frequency (150–200 Hz) by a piezoelectric actuator in solution ~1 tip ball distance from the sample surface. If an electric current is present due to ion flux, the electric charge on the platinum ball fluctuates in proportion to the size of the current. The probe is connected to a lock-in amplifier (Stanford Research Systems, model SR530) that locks on to the probe’s specific frequency. The probe is calibrated with a set current density of 1.5 µA/cm2 at the start and end of experiment. Before measurements, the probe is vibrated in solution far from the sample ( > 1 cm), where there is no electric current, to establish a baseline. The probe is then moved into measuring position close and parallel to the sample surface, with the vibration direction perpendicular to the sample surface (see Fig. 1a). Measurements on different stages of chicken embryos were done at room temperature in chick Ringer’s solution containing (mM): 148 NaCl, 5.6 KCl, 1.1 CaCl2.6H20, 1 MgCl2.6H20, 5 HEPES, pH adjusted to 7.0 with NaOH.

Retrovirus preparation and injection

RCAS-β-Catenin and RCAS-SHH have been reported previously16,64. To construct RCAS-GCaMP6s-T2A-mCherry, the GCaMP6s sequence was amplified from a CMV-GCaMP6s vector (Addgene # 40753), then digested with NotI, SpeI and subcloned into an RCAS(B)-T2A-mCherry vector. To construct RCAN-GBS-GFP vector, GBS-GFP was amplified from a pBS-KS vector from Dr. Briscoe (The Francis Crick Institute, UK), then digested with ClaI and subcloned into an RCAN vector. To construct RCAS-mCherry-LOV-cSTIM1, we first replaced the mouse STIM1 fragment (amino acid 336–486) in the original construct32 with the corresponding chicken sequence amplified. Next the whole mCherry-LOV-cSTIM1 cassette was amplified with attB primers. The PCR fragment was subcloned into RCAS-DV (Addgene # 11478) using gateway recombination reactions. To construct the lentiviral vector expressing shRNA against Connexin-43, we designed the shRNA target sequence using Block-iT RNAi designer. The annealed primers were cloned into the pLL3.7 vector from Addgene (11795)34. Virus packaging was done in HEK293T cells with pCMV-VSVG and pCMV-dR8.2. Both RCAS and lentivirus were concentrated by ultra-centrifuging in a BECKMAN Coulter L8–80M (SW28 rotor) at 26000 rpm for 1.5 h. Concentrated viruses were injected into somites of H&H 14 or 17 chicken embryos. Primers used for subcloning are listed in Supplementary Table 2.

Embryonic chicken skin explant/strip and cell culture

For chicken skin explant cultures14, dorsal skins from chicken embryos at corresponding stages were dissected in Hank’s buffered saline solution and the explants were transferred to culture inserts (Falcon, 0.4 μm pore) for imaging. For making strips, the explants were transferred to PELCO glass-bottom dishes (50 × 7 mm) coated with 1 mg/ml Poly-L-lysine (Sigma, P6282) and Fibronectin (Sigma, F1141). After they fully attached the explants were examined under fluorescent microscope and the regions highly infected by RCAS-GCaMP6s-2A-mCherry virus were cut into one-bud-wide strips. The strips were placed in coated glass-bottom dishes on their sides for imaging. For dissociated mesenchymal cell culture, the epithelium and mesenchyme of embryonic chicken dorsal skins were separated by 20 min incubation in 2x CMF. The mesenchyme was dissociated by 0.35% type I collagenase treatment for 20 min. The digestion was stopped by the addition of FBS and the cells were seeded into culture dishes. Chemicals used in tissue culture: Nifedipine, Nitrendipine, Carbenoxolone disodium, 18-α-GA, Lanthanum chloride, Lithium chloride and Mefloquine were purchased from Sigma-Aldrich. N-[4-[3,5-Bis(trifluoromethyl)-1H-pyrazol-1-yl]phenyl]-4-methyl-1,2,3- thiadiazole-5-carboxamide (BTP2), [(3aR*,4 S*,7 R*,7aS)-1,3,3a,4,7,7a-Hexahydro-1,3-dioxo-4,7-methano-2H-isoindol-2-yl]-N-8-quinolinylbenzamide (endo-IWR1), Phorbol 12-myristate 13-acetate (PMA), 3-Chloro-N-[trans-4-(methylamino)cyclohexyl]-N-[[3-(4-pyridinyl)phenyl]methyl]benzo[b]thiophene-2-carboxamide (SAG), and Thapsigargin were purchased from Tocris. Cyclopamine was purchased from LC Laboratories. Recombinant mouse Shh N-terminal peptide was purchased from R&D Systems. Feather bud aspect ratio (Major Axis/minor Axis) was calculated in ImageJ by using freehand or ellipse selection tool to mark the contour of feather buds.

Characterization of cell proliferation and apoptosis

Two hours before skin explants were collected and fixed in 4% PFA, 10 μl 1% BrdU (Sigma) were added to the culture media to label the proliferating cells. After fixation (4 °C overnight), samples were dehydrated in alcohol, cleared in Xylene, and then embedded in paraffin. The paraffin blocks were cut into 8 μm sections. Before staining for BrdU (Abcam ab6326 1:200 dilution), the sections were incubated in 10 mM Citrate buffer (pH = 6.0) at 95 °C for 0.5 h. Secondary antibody was anti-Rat-Alexa 488 (Thermo Scientific). To detect apoptotic cells we employed the TUNEL kit (Sigma 11684795910) and followed the protocol with proteinase K treatment (10 μg/ml for 15 min at room temperature).

Time-lapse Ca2+ imaging in cultured skin under perfusion

H&H 34 or 35 embryonic chicken dorsal skin explants were cultured on a rectangular PET membrane (cut from Fisher Scientific 6-well cell culture insert) placed on two spacers in a WillCo 35 mm glass-bottomed dish (skin strips were directly put on coated glass-bottomed dish) for perfusion experiments. The culture media is DMEM (without Phenol red) containing 10% FBS, 2% chicken serum and 10 mM HEPES. Right before imaging, the culture media was replaced by Ringer’s solution. The custom-built recording chamber was placed on a Zeiss Pascal confocal microscope with a 40 × /0.8 NA water immersion objective, and the chamber was warmed to 38.5 °C. Solenoid valve-controlled four barrel perfusion system was set up on the recording chamber, and the average flow rate of bath perfusion was about 1.4 ml/min. Due to the bath perfusion configuration, solution exchange was slow and was completed within 2 min.

Time-lapse Ca2+ imaging of dissociated cells

Dissociated H&H 31 or H&H 35 embryonic skin mesenchymal cells were cultured on 0.01% poly-L-ornithine coated-glass chips (0.5 × 0.5 cm). The mixture of 4 µM AM-Fura-2 Ca2+ dyes (Life Technologies) and 0.04% pluronic F-127 (Sigma) were loaded in the presence of Ringer’s solution for 25 min in a 37 °C CO2 incubator. After washing with Ringer’s solution for 10 min, each glass chip was placed onto a recording chamber equipped with a local perfusion system. The custom-built local perfusion system was placed right next to a field of view and was able to exchange each test solution with a time constant of 100 ms65. An inverted Axiovert 100 microscope (Zeiss) was used and equipped with a monochromator (Polychrome V; TILL Photonics) to generate 350 nm and 380 nm excitation wavelength for Fura-2. Each excitation wavelength was illuminated for 200 ms at 1 Hz sampling frequency through a 63 × /0.9 NA achroplan water immersion objective. The corresponding emission intensity was detected with a 16-bit depth EMCCD camera (iXon Ultra 897, Andor Technology) operated by MetaFluor (Version 7.8, Universal Imaging). All recordings were done at room temperature. For ROI analysis, background-subtracted intensity traces were imported into IGOR Pro 6.22 A (Wavemetrics), and analyzed using custom-written data analysis routines. For testing activities of the chicken version of the opto-cCRAC construct, Hela cells were transfected with 300 ng plenti-mcherry-LOV-cSTIM1 and 300 ng pGP-CMV-NES-jRCaMP1b (addgene#63136) in 35 mm glass-bottom dishes. Sixteen hours post-transfection, cells were recorded under 594 nm channel: 30s-off, followed by two cycles of on (blue light 1 min) and off (2 min).

Solutions used for time-lapse Ca2+ imaging

The skin explants expressing RCAS-GCaMP6s-T2A-mCherry were washed with 2 mM Ca2+ Ringer’s solution containing (mM): 140 NaCl, 2.8 KCl, 10 HEPES, 1 MgCl2, 2 CaCl2, and 10 D-glucose (pH 7.2 adjusted with 1 N NaOH, 290~ 300 mOsm adjusted with D-glucose). 100 mM KCl solution was composed of 100 KCl, 50 NaCl, 10 HEPES, 1 MgCl2, 2 CaCl2, and 10 D-glucose (pH 7.2 adjusted with 1 N KOH, 290~ 300 mOsm adjusted with D-glucose). Ca2+ free solution was composed of 140 NaCl, 2.8 KCl, 10 HEPES, 1 MgCl2, 1 mM EGTA, and 10 D-glucose (pH 7.2 adjusted with 1 N NaOH, 290~ 300 mOsm adjusted with D-glucose). All the solutions were filtered using bottle-top filters with a 0.2 μm pore size membrane before use.

Patch clamp experiment for VGCC current recording

Dissociated mesenchymal cells from H&H 35 embryonic chicken skins were cultured on collagen-coated-glass chips (rat tail type I collagen, Sigma). Internal solution was composed of (in mM) 120 CsGlutamate, 10 HEPES, 2 MgATP, 0.3 Na2GTP, 10 NaCl, 10 EGTA, and 10 TEACl (pH 7.2 adjusted with 1 N CsOH, 290 mOsm). The internal solution was filled into fire-polished glass pipettes prepared using a PC-10 patch pipette puller (Narishige, Japan). Pipette resistance ranged from 4.5 Mohm to 5.5 Mohm. The cells were placed on a recording chamber and washed with 2 mM Ca2+ Ringer’s solution. An inverted Axiovert 100 microscope (Zeiss) with a 63 × /0.9 NA water immersion objective was used to locate single mesenchymal cells. After forming a gigaohm seal between a patch pipette and cell plasma membrane, a standard whole-cell configuration was prepared using an EPC9 amplifier (HEKA Elektronik, Germany). Pipette capacitance and membrane capacitance were compensated and further eliminated using a P/4 protocol during current recordings. Series resistance ranged from 10 Mohm to 20 Mohm. A step voltage protocol written using PatchMaster Version 2 × 73.5 was applied to voltage-clamped cells. Currents were filtered at 2.5 kHz using a 4-pole bessel filter and digitized at a sampling frequency of 10 kHz. For data analysis, current traces were imported into IGOR Pro 6.22 A (Wavemetrics), and current-voltage plots were generated using a custom-written data analysis routine.

4D Ca2+ imaging and cell nucleus imaging

H&H 34 chicken dorsal skins were cultured for 3–4 h before imaging in a Fisher Scientific 6- well culture insert (upper wall trimmed) mounted on 4 spacers glued to a WillCo 50 mm glass-bottom dish with 3 ml culture media underneath it. Right before imaging 1.8 ml culture media was added on top of the skin. A non-lubricated condom was used to make a sealed chamber between the dish and the microscope lens. Both the lens and the dish were warmed for 1.5–2 h before imaging. For 4D ratiometric Ca2+ imaging in skin explants, the interval between z-stack scans was 6 min (scanning time was ~ 2 min). The interval was 1.5 min for skin strips. For 4D nuclear imaging, the interval was 3 min (~ 1 min scanning time). 3D rendering, cell tracking was done in IMARIS (Bitplane). Segmentation of the feather mesenchyme, ROI analyses were done in ImageJ. Quantification of movement patterns and generation of pseudocolor images were done in MATLAB. The duration of the slow Ca2+ transients were determined by measuring the time interval between the peaks or valleys on the F GCaMP6s/F mCherry ratio plots. To calculate the spreading speed of the multicellular Ca2+ transients, the frontiers of the wave propagation were manually determined in the psendo-color images at different time points and the distances between the frontiers were measured and divided by the time intervals.

Photo-activation of opto-cCRAC in cultured cells and skin

For the cultured mesenchymal cells, concentrated RCAS-mCherry-LOV-cSTIM1 virus was added to cell culture media (1:200) for 48 h. The cells were loaded with the Ca2+ indicator AM-Fluo-4 plus pluornic F-127 (Thermo Fisher) for 30 min and then washed with HBSS (no Phenol Red) before imaging. Imaging was done in a Zeiss LSM510 confocal microscope at 38 °C. For the skin culture, skins from H&H 31 embryos injected with the virus (only to the left body side) were cultured on a culture insert for 48 h within a black WillCo dish with a hole on top to insert LED light. Photostimulation was provided by an external blue light (470 nm, at roughly 20 mW/mm2, ThorLabs Inc., Newton, NJ, USA). Light cycles (2 min on/off) were applied by programming DC2100 LED Driver with LabVIEW (National Institute). Measurement of feather aspect ratios were calculated in ImageJ by using the elliptical selection tool to mark feather contour.

RNA-Seq and ChIP-Seq

Skins dissected from H&H 31 and H&H 35 chicken embryos were used for RNA-Seq and ChIP-Seq library preparation. For RNA-Seq epithelial and mesenchymal tissues were separated in 2X CMF (calcium-magnesium free saline). Total RNA was extracted using Trizol reagent. For library construction we used TruSeq RNA Sample Prep Kit Version2 (Illumina). Two biological replicates were sent for sequencing (50 bp, single end) with Illumina HiSeq 2000 in the USC Epigenome Center. FastQ files were trimmed and mapped to the chicken genome (galGal4) using Partek Flow. Further analysis was done in Partek Genomic Suite. For the ChIP-seq experiments66, embryonic skin were dissociated by 0.35% collagenase (type I) digestion before formaldehyde cross-linking. Sonication time was 20 min (30 sec on/off cycle). H3K4me3 antibody came from Abcam (ab8580, lot GR188955-1). IgG and input DNA were used as background controls. Biological replicates were sent for library preparation and sequencing by the USC Epigenome Center. Reads were trimmed based on quality and aligned to galGal4 in Galaxy. Peak calling was done with QuEST39. For motif search we applied TRANSFAC (BIOBASE), with the cut-off condition set to minimize false positives.

In situ hybridization and immunostaining

In situ hybridization and immunostaining were done as previously described14. Primers used for cloning in situ probes are listed in Supplementary Table 2.

Primary antibodies for immunostaining: β-Catenin (Sigma, 15b8); Connexin-43 (Santa Cruz Biotechnology, sc-9059); BrdU (ABCAM, AB6326); GFP (NOVUS, NB600-308); LCAM (Chuong and Edelman. 1985); Neurofilament (3A10, DSHB); VIM (H5, DSHB). Secondary antibodies were labeled with Alexa Fluor 488 or 546 (Thermo Fisher).

RT-qPCR for skin and cultured mesenchymal cells

RNA extraction was done with Zymo Research Direct-zol RNA Kits. Reverse transcription was done using Superscript III First Strand Synthesis kit. The RNA and cDNA concentrations were measured with the NanoDrop 2000 spectrophotometer and normalized between samples. Primers used for qPCR are listed in Supplementary Table 2. The Ct values were measured using the Agilent Mx3000P qPCR system. The relative quantification was done by pyQPCR Version 0.9 software.

Scrape-Load dye transfer assay

Dorsal skins of H&H stage 30 and 33 chicken embryos were peeled off and cultured on 6-well culture inserts for 1 day till they reached the proper developmental stages. Control, 18-α-GA, or PMA-treated skins were covered with 2 mg/ml Lucifer Yellow (Sigma) and 1 mg/ml Rhodamine–Dextran (Thermo Fisher) dissolved in HBSS when the feather buds were cut by Tungsten needles. Dyes were rinsed off after 5 min and the skins were washed two more times. Images of the scraped feather buds were taken 8–10 min after dye loading.


In order to test whether datasets were normally distributed random samples, the Kolmogorov–Smirnov tests were conducted. Two independent sample T-tests were used for comparing unpaired sample groups. For some datasets not equally and normally distributed, Wilcoxon rank tests were conducted using IGOR Pro or MATLAB to evaluate statistically significant difference between two samples. Chi-square test was conducted in MATLAB. To evaluate whether the directionality of migrating mesenchymal cells (circular dataset) had significant differences in different experimental conditions, Watson’s U2 tests were conducted in MATLAB.