Sensory axons must traverse a spinal cord glia limitans to connect the brain with the periphery. The fundamental mechanism of how these axons enter the spinal cord is still debatable; both Ramon y Cajal’s battering ram hypothesis and a boundary cap model have been proposed. To distinguish between these hypotheses, we visualized the entry of pioneer axons into the dorsal root entry zone (DREZ) with time-lapse imaging in zebrafish. Here, we identify that DRG pioneer axons enter the DREZ before the arrival of neural crest cells at the DREZ. Instead, actin-rich invadopodia in the pioneer axon are necessary and sufficient for DREZ entry. Using photoactivable Rac1, we demonstrate cell-autonomous functioning of invasive structures in pioneer axon spinal entry. Together these data support the model that actin-rich invasion structures dynamically drive pioneer axon entry into the spinal cord, indicating that distinct pioneer and secondary events occur at the DREZ.
The somatosensory nerve detects sensory stimuli in the periphery and relays the information to the central nervous system (CNS)1,2,3. To ensure sensory information is rapid and uninterrupted, glial cells and axons coordinate at the dorsal root entry zone (DREZ), the CNS/peripheral nervous system (PNS) interface where sensory axons establish their dual domain nature4,5. During development, these sensory axons of the dorsal root ganglia (DRG) traverse into the spinal cord and glial cells reorganize6,7. This strict organization of the nerve is essential to drive somatosensory-induced behavior.
Our understanding of sensory nerve assembly and how numerous cell types dynamically interact during it are predicated on studies that have shown that ingrowth of sensory axons into the spinal cord occurs as neural crest cells are docked at the DREZ7. In contrast, Ramon y Cajal’s observation of pioneering 8th ganglion growth cones in developing otocyst presented a battering ram model where the growth cone employed an amoeboid mass to navigate through tissue with high cellular density8. Whether the battering ram is a distinct axonal structure or an overall term for the growth cone is unclear. Time-lapse imaging of pioneer axons shows that neural crest cells associate with the axons while they navigate to the DREZ, but the growth cone leads the neural crest cells6. In such imaging, however, the actual entry of the axons was not investigated. The temporal order of cellular assembly at the DREZ and whether there are distinct pioneer and secondary events, therefore, remains an unclear but critical question.
Classically, filopodia and lamellipodia have been described as the major motile structures in extending growth cones that aid navigation. Recently, other structures like invadopodia which are best understood in cancer cells as a method of cellular invasion and metastasis9 have been added to the repertoire of axon guidance structures10. These invadopodia impressively form in axons across phylogeny10. These data further demonstrate striking invadopodia morphology in growth cones and that invadopodia-related molecules are essential in motor axon navigation10; however, control of invadopodia in dynamic concert with classical growth cone machinery at specific anatomical decision points remains elusive. How the underlying dynamics drive growth cone machineries within distinct cellular milieu therefore remain unlinked and unexplored. These potential links could provide a step-wise blueprint for DREZ assembly.
Here, we used time-lapse imaging of pioneer axons in zebrafish to understand how pioneer sensory neurons dynamically grow into the spinal cord. We visualize the first axons crossing the glia limitans into the spinal cord. We first identify that neural crest boundary cells are absent from the DREZ during pioneer axon entry into the spinal cord. Without boundary cap cells to provide a substrate for ingrowth, actin-rich invasive structures, reminiscent of invadopodia, form in the growth cone. We then show invasion structures are essential for pioneer axons to enter the spinal cord. Using laser-induced lesions of the spinal tissue to mimic spinal cord breach, we demonstrate that we can bypass the necessity of invasive structures during axonal entry. Therefore, spinal ingrowth of the pioneer sensory axon is dependent on changing growth cone morphologies that invade into the spinal cord. We propose a modified model that invasive structures and boundary cap cells are both used by DRG axons but are temporally segregated by pioneer and secondary events.
Neural crest cells are absent from DREZ during pioneer ingrowth
Dorsal root ganglia neuronal ingrowth has been proposed to depend on neural crest cells that sit at the DREZ7. To test their role in DRG pioneer axon entry we used zebrafish to visualize their localization. At 48 h post fertilization (hpf), the DRG consists of a single neuron with a soma ensheathed by Sox10+ glia (Fig. 1a)11. Between 48 and 72 hpf, zebrafish dorsal root ganglia pioneer axons initiate dorsally, navigate to the DREZ, and cross into the spinal cord6,11. The DREZ is established 18.075 ± 0.681 µm (mean ± SEM) from the DRG neuronal soma (Fig. 1a, b). To test if boundary cap cells interact with the pioneer axon, we first used Tg(ngn1:gfp) animals to mark DRG neurons and stained for the neural crest cells with Sox10 at 56 hpf12. DRG development occurs in an anterior to posterior fashion. As a result, at 56 hpf the anterior-most DRG neurons (DRG ~1–10) have entered the spinal cord, the middle-located DRG (DRG ~11–20) are at or approaching the DREZ, and the posterior-most (DRG ~20–32) have not entered. This time point provides a developmental gradient of pioneer axon entry. In the ganglia, GFP+ neuronal cell bodies in both the anterior and posterior associated with ~3 Sox10+ cells. However, Sox10+ cell bodies were not present at the DREZ during these initial pioneer phases (Fig. 1c, d, n = 25 DRG). The localization of Sox10+ cells around the neuronal somas was evident when we measured the dorsal-most Sox10+ glia to the DREZ to be 14.46 ± 0.670 µm (Fig. 1a, b), consistent with soma-ensheathing glia11,13. These data, however, are inconsistent with the presence of a mature boundary cap population.
We next hypothesized that neural crest processes contact the DREZ before the pioneer axon14. To test this, we time-lapse imaged pioneer axon navigation in Tg(ngn1:gfp); Tg(sox10:gal4); Tg(uas:mcherry) animals by generating z-stacks of DRG every 5 min for 24 h starting at 48 hpf15,16. In these images, the pioneer axon appears yellow because of co-expression of mCherry and green fluorescent protein (GFP), and the glia appear red due to mCherry expression only. Initially, the pioneer axon and associated glia extend together (Fig. 1e, f). However, before the axon contacts the DREZ during entry the mCherry+ glia trail the growth cone, and when the axon reaches the DREZ, most of the axon is not associated with any glia (Fig. 1e, f). Following axon entry at the DREZ, glia continue navigation toward the DREZ (Fig. 1e, f). However, in these movies the glia only contacted the DREZ following axon spinal cord entry (Fig. 1e, f).
To further confirm this observation, we used Tg(sox10:eos) animals which express Eos protein in DRG cells17. With these animals, we could label single DRG cells by selectively exposing a specific 8 µm region to ultraviolet light, causing Eos fluorescent photoconversion18. At this stage in development, the DRG consists of only 3–4 cells (ensheathing glia and 1 neuron), allowing us to reliably photoconvert single DRG neurons before pioneer axon initiation while minimizing off-target effects11,18. After conversion, we created movies of pioneer axon navigation to the DREZ by collecting images every 5 min for 24 h. Cell tracings of these movies showed that the photoconverted pioneer axon contacted the DREZ before the non-photoconverted glia in 89% of our movies (Fig. 1g, Supplementary Figure 1a). Specifically, the pioneer axon contacts the DREZ 146.1 ± 41.21 min before glial DREZ contact (Fig. 1h, n = 9 DRG, p = 0.0076, paired Student’s t-test).
To rule out the possibility that thin, glial extensions that are not labeled with cytosolic markers contact the DREZ before neurons, we expressed membrane-tagged enhanced GFP (meGFP) under the ngn1(−3.1 kb) promoter in Tg(sox10:mrfp) animals, which express membrane-tagged red fluorescent protein (mRFP) in all DRG cells19. In these animals, neuronal membranes are labeled with meGFP and mRFP to appear yellow, and glial membrane is labeled only with mRFP to appear red. Time-lapse images of DRG pioneer axons in these animals clearly show that yellow membranous processes from the pioneering growth cone contact the DREZ before the glial cell membrane (Supplementary Figure 1b). The totality of these complementary data are inconsistent with a model that pioneer axon ingrowth at the DREZ is dependent on neural crest cells.
Pioneer axons change morphology during spinal cord entry
Before the description of boundary cap cell populations, Ramon y Cajal described the appearance of amoeboid battering ram structures in developing axons8. To explore this possibility, we visualized the pioneer axon using Tg(sox10:mrfp) animals and radial glial cells that represent the glia limitans at the DREZ by expressing GFP with gfap regulatory sequences, Tg(gfap:gfp)20. At 48 hpf, the radial glial boundary separates the DRG cells from the spinal cord, and by 72 hpf, mRFP+ DRG axons have crossed the radial glia and formed anterior/posterior projections in the CNS (Fig. 2a). To understand how this cellular arrangement occurred, we expanded this analysis by visualizing the pioneer axon and radial glia every 5 min for 24 h during navigation into the CNS (Supplementary Figure 2a, Supplementary Movie 1). In these movies, the pioneer axon navigated along the radial glial boundary on the PNS side, then crossed the CNS/PNS radial glial boundary and formed anterior and posterior projections in the CNS (Fig. 2a). Before and after crossing of the glia limitans, the pioneer axon growth cone appears thin and finger-like (Fig. 2b). However, during entry the growth cone swells with a large amount of cytosol at its tip, reminiscent of Cajal’s description of a battering ram21 (Fig. 2b). Multiple growth cone swellings have been described including collapsed growth cones (in development), retraction bulbs, and dystrophic endings (in regeneration)22,23. We next sought to compare the growth cone structure at the DREZ to these structures using Tg(sox10:mrfp) animals. We visualized a collapsed growth cone as a DRG neurite retracted to the cell soma after it failed to specify as the single DRG axon. These images revealed a membranous flare at the growth cone tip, consistent with previous reports of retraction bulbs23 (Supplementary Figure 2a). We also tested if the growth cone structure at the DREZ was like a retraction bulb/dystrophic ending in a regenerative context by axotomizing spinal axons. Following injury, the spinal axon formed a spherical bulb lacking any projections (Supplementary Figure 2a), consistent with previous reports of retraction bulbs and dystrophic endings but distinct from the growth cone structures at the DREZ22. These data are consistent with the hypothesis that a unique growth cone structure is dynamically employed at the DREZ.
To confirm these morphological changes in the pioneer axon occurred during axonal crossing of the radial glial membrane, we quantified intensity profiles of Tg(gfap:gfp) and Tg(sox10:mrfp) along the glia limitans (y-axis) and through the growth cone (z-axis) as outlined in Fig. 2c. These intensity profiles demonstrated a decrease in Tg(gfap:gfp) intensity during entry (Fig. 2d, e). Following entry, the mRFP+ growth cone was localized medial to the glia limitans (Fig. 2d, e). As further confirmation of this entry event, we quantified the intensity of Tg(gfap:gfp) at the DREZ during the navigation of the Tg(sox10:mrfp)+ pioneer axons into the spinal cord. To do this we used tracking software to trace the intensity of GFP at the DREZ during entry. Single tracings of these data indicate that Tg(gfap:gfp) intensity at the DREZ decreases as the axon enters (Supplementary Figure 2b-d, n = 7 DRG, p = 0.0128). Dynamic Tg(gfap:gfp) intensity was also evident in other areas of the spinal cord but the Tg(gfap:gfp) intensity at the nascent DREZ was consistently decreased during pioneer axon spinal cord entry. To test this further, we measured the intensity of Tg(gfap:gfp) at the DREZ when pioneer axon entry into the spinal cord fails (as shown below). These measurements revealed no difference in Tg(gfap:gfp) intensity at the DREZ before and after failed axon entry into the spinal cord (Supplementary Figure 2e, f, p = 0.7742, n = 5 DREZ, Tukey’s HSD (honestly significant difference). Together, these data support the hypothesis that pioneer axons cross a radial glial membrane boundary by either penetrating that boundary or causing its rearrangement.
To understand the dynamics of this enlarged growth cone structure, we next traced the location of the pioneer growth cone during and after its navigation to the DREZ. These tracings revealed it formed during stalling of the pioneer axon at the DREZ (Fig. 2f, g, n = 4 axons). Following entry and disassembly of the growth cone structure at the DREZ, the axon sped back up, continuing its navigation.
To rule out that this stalling phenomenon is the pioneer axon waiting for glial arrival at the DREZ, we measured that stalling lasted at most 100 min following initial DREZ contact. Our data in Fig. 1e demonstrate that glial arrival at the DREZ occurs ~146 min after axon DREZ contact (Fig. 2g), arguing strongly against this hypothesis. Instead, these data are consistent with a model where the pioneer axon navigates dorsally using filopodia, stalls specifically at the DREZ to reorganize into a unique structure, and returns to filopodial navigation following entry.
Actin-rich structures form at the DREZ
In cancer, actin-rich invasion structures have been shown to be fundamentally important for cells to cross cellular boundaries9. Similar structures have also been recently shown to form in freely navigating axons grown in cell culture conditions and have been implicated in motor axon navigation10. We hypothesized that pioneer axon crossing into the spinal cord could utilize these invasive structures. We therefore visualized actin dynamics with Lifeact-GFP24, a marker for F-actin that does not perturb its dynamics, under sox10 regulatory sequences, Tg(sox10:gal4); Tg(uas:lifeact-gfp)24. In time-lapse movies of pioneer axon navigation, the growth cone exhibited filopodia-like extensions before it reached the DREZ (Fig. 3a, Supplementary Movie 2). At the DREZ, Lifeact-GFP concentrated within the center of the growth cone, and most filopodial extensions retracted. This concentration of Lifeact-GFP dispersed as the axon returned to a filopodia-like morphology (Fig. 3a–c). The dynamic concentration of Lifeact-GFP corresponded with the swollen growth cone morphology at the DREZ. Intensity measurements of growth cone Lifeact-GFP show a distinct increase while at the DREZ (n = 6 DRG, p < 0.0350, Tukey’s HSD) (Fig. 3b, c). We next asked where in the growth cone the Lifeact-GFP concentration is present (e.g., tip of growth cone, center of growth cone, base of growth cone). To do this we quantified the distance of the actin concentration to the center of the growth cone. In this quantification, we measured that while at the DREZ, the Lifeact-GFP concentrate filled the growth cone center. Meanwhile, before and after entry the most intense concentration localized in the growth cone tips where the filopodia were present (n = 6 growth cones, p < 0.0001, Tukey’s HSD) (Fig. 3d). Actin-rich invasive structures have been shown to form basally projecting formations. We, therefore, used deconvolution software to determine if Lifeact-GFP concentrates were basally projecting. In this analysis we identified that while at the DREZ, Lifeact-GFP puncta exhibited thin basally projecting Lifeact-GFP structures (Fig. 3e). In contrast, the filopodia-like extensions that occurred before and after entry were not basally projecting. Together, these data support the hypothesis that pioneer axons dynamically reorganize their actin from filopodia into basally projecting concentrates specifically at the DREZ.
Actin-rich structures cross the radial glia membrane
To test if these actin-rich structures are employed to cross the glia limitans, we time-lapse imaged actin in DRG neurons with Lifeact-GFP in an animal that also expressed mCherry in radial glia, Tg(gfap:nsfb-mcherry)25,26 (Fig. 3f, Supplementary Movie 3). Single planes of the CNS/PNS boundary revealed a reduction of mCherry intensity within radial glia during Lifeact-GFP rearrangement at the DREZ, suggesting that actin-rich structures could be utilized to cross the glia limitans (Fig. 3g, h, n = 8 DRG). We further tested this hypothesis with measurements of different axes as in Fig. 2c (Supplementary Movie 4). Before entry, Lifeact-GFP was present along a coherent gfap+ border in the y-plane and overlaid with the gfap+ peak in the z-plane before entry, suggesting that pioneer axons navigate along the radial glial boundary (Fig. 3i, j). During DREZ entry, the Lifeact-GFP intensity increases and the gfap intensity decreases to nearly zero (Fig. 3i, j). After the axon has entered, the gfap+ glia limitans peak is lateral to the Lifeact-GFP peak in the z-plane (Fig. 3i, j). These results are consistent with the hypothesis that actin-rich structures dynamically rearrange specifically to cross the glia limitans.
Actin-rich structures form to cross a radial glial boundary
If actin-rich structures form to cross a radial glial membrane at the DREZ, then an incoherent DREZ boundary should render actin concentrates dispensable. To test this possibility, we created focal lesions in the radial glial at the DREZ. We first sought to test the feasibility of this paradigm using a diffraction-limited high-energy pulsed laser (Ablate©) to create a 12–14 µm size aberration in the spinal cord in Tg(gfap:gfp); Tg(sox10:mrfp) animals. Lesions were created at two DREZ per animal, and adjacent nerves in the imaging window were used as non-lesion controls (Fig. 4a). To confirm the specificity of the lesion, we digitally rotated these images 90 degrees across a single y-plane to visualize the lesion size at different spatial areas (Fig. 4a). In planes 15.9 µm away from the lesion, the glia limitans was indistinguishable from adjacent non-lesioned DREZ (Fig. 4a). To ensure that the lesion did not induce excessive damage to surrounding tissue we visualized overall tissue integrity with transmitted light. With transmitted light, damage surrounding the lesion was minimal (Supplementary Figure 3a, b). To rule out the possibility that the ablation only photobleached the glia limitans, we also visualized a loss of glial fibrillary acidic protein (GFAP) via immunohistochemistry (Supplementary Figure 3c). Next, we confirmed that axons approaching a lesioned DREZ were entering the spinal cord by digitally rotating the images of the axons after entry 90 degrees (Fig. 4a). In doing so, a clear mRFP+ intensity from the DRG axons is medial to the gfap+ boundary, supporting the conclusion that these axons entered the spinal cord (Fig. 4a).
We then created lesions in Tg(sox10:lifeact-GFP); Tg(gfap:nsfb-mcherry) animals at 48 hpf at the DREZ before the axons had reached the DREZ, then imaged z-stacks for 24 h (Fig. 4b, Supplementary Movie 5). In non-lesioned nerves, all pioneer axons produce actin-rich structures at the DREZ and enter the spinal cord (n = 8 DRG). In lesioned nerves, 33% of the pioneer axons produced actin-rich formations at the DREZ but all axons entered the spinal cord (n = 9 DRG) (Fig. 4c). We confirmed that the DREZ region was lesioned by scoring mCherry intensity and detected a decrease at lesioned DREZ (n = 8 non-lesioned, n = 9 lesioned, p < 0.0001, Tukey’s HSD) (Fig. 4d). We also observed no changes in the formation of anterior and posterior axonal projections inside the spinal cord across the treatment groups (Supplementary Figure 3d).
To characterize axon navigation in this paradigm, we traced pioneer axons during navigation in these movies and observed an absence of growth cone morphological changes as the axons approach the lesioned DREZ (Fig. 4e, Supplementary Figure 3e). Further, axons with lesioned DREZ displayed shorter actin concentrations (n = 9 lesioned, n = 8 non-lesioned, p = 0.0216, Tukey’s HSD) (Fig. 4f). In the few cases where actin concentrates did form, they initiated prematurely, indicating they entered in more ventral locations than the DREZ lesion (n = 9 lesioned, n = 8 non-lesioned, p = 0.0012, Tukey’s HSD) (Fig. 4g). We confirmed that pioneer axons entered the spinal cord in both the lesion and non-lesion conditions by digitally rotating images of the DRG and detecting the Lifeact-GFP+ axon inside the mCherry+ glia limitans (Fig. 4h, i). These data are consistent with the hypothesis that actin-rich structures form to breach a radial glial boundary and in the absence of such a boundary, actin-rich formations are dispensable.
Perturbation of actin concentrates disrupts axon entry
If actin-rich structures are employed in the growth cone to cross the glia limitans, then disrupting them should perturb entry of axons into the spinal cord. The requirement of invasion components in precursor events to DREZ formation prevented the use of genetic mutants to test their requirement at the DREZ27. Therefore, we first tested bioactive molecules shown to alter actin-rich invasion structures. We identified two molecules that had strong opposite effects on the actin-rich structures that form in pioneer axons at the DREZ9,10,27,28. SU6656 disrupted the formation of actin concentrates in pioneer axons (Fig. 5a, b, Supplementary Figure 4a). SU6656 inhibits Src family kinases which promote the formation of invadopodia, an important mechanism of cancer cell invasion9,28. SU6656 is highly selective for Src kinases compared to other protein kinases29. Paclitaxel, which stabilizes microtubules by direct binding and has been shown to promote invadopodia formation, increased the duration of actin concentrates in pioneer axons (Fig. 5a, b)28. Differences in the morphologies of DRG and their axons were indiscernible across treatments (n = 14 dimethyl sulfoxide (DMSO); n = 20 SU6656; n = 13 paclitaxel) (Supplementary Figure 4b-d). Similarly, no significant defects in gross morphology of treated animals were detected (Supplementary Figure 4e).
We next tested if treatment of SU6656 perturbs actin-rich invasion component formation. To do this we treated animals with SU6656 at 36–72 hpf, after neural crest migration is completed17. We then imaged z-stacks of Tg(sox10:lifeact-GFP) animals every 5 min for 24 h starting at 48 hpf (Fig. 5a, Supplementary Movie 6). Measurements of Lifeact-GFP peak during navigation revealed an abrogation of the actin peak (Fig. 5b, n = 10 DMSO-treated, n = 14 SU6656-treated), and only 60% of SU6656-treated axons produced actin concentrates and 55% entered the spinal cord (n = 20 DRG) (Fig. 5c). All SU6656-treated axons that entered the spinal cord formed actin concentrates, supporting the hypothesis that invasion components are essential to enter the spinal cord (n = 20 DRG) (Fig. 5c). As confirmation that Src inhibition reduces stability of invasive structures, we scored that SU6656-treated pioneer axons formed actin peaks later than control animals (n = 14 treated DRG, n = 14 untreated DRG, p = 0.0298, Tukey’s HSD) (Supplementary Figures 4f-h).
To further test if invasion components are required to cross the DREZ, we tested additional bioactive molecules that disrupt cell invasion28. We identified that Cdk inhibitor Purvalanol A, MEK inhibitor U0126, and pan-MMP inhibitor GM6001 also disrupt axon entry. Treatment with these drugs at 36 hpf phenocopied entry deficits of SU6656 treatment (Fig. 5c, Supplementary Figure 4i). We did not visualize differences in DRG number, axon initiation defects, or deficiencies in navigation to the DREZ in these treatments (Supplementary Figures 4b-d). It should be noted that GM6001 can also inhibit other zinc-dependent proteinases and U0126 has been shown to prevent calcium transients in some cells30,31. Purvalanol A is specific to Cdk family members32. Taken together, these complementary data support the hypothesis that actin-rich invasion components are required to enter at the DREZ.
Invasion components are sufficient for spinal cord entry
If invasion components are sufficient to cross the radial glia boundary at the spinal cord, then their formation before axon arrival to the DREZ should result in premature axon entry. To test this, we treated Tg(sox10:lifeact-GFP) animals at 36 hpf with paclitaxel, a molecule known to stabilize invadopodia (Fig. 5b)28 and time-lapse imaged those animals for 24 h starting at 48 hpf (Fig. 5a, Supplementary Movie 7). To confirm that paclitaxel impacts actin-rich invasion components in DRG pioneer axons, we measured Lifeact-GFP intensities in animals treated with paclitaxel and quantified an increase in the duration of actin concentrates (n = 13 paclitaxel-treated, n = 14 DMSO-treated, p = 0.0001, Tukey’s HSD) (Supplementary Figure 4h). These invasion components also formed earlier in the axon’s navigation (Fig. 5b, n = 10 DMSO-treated, n = 14 paclitaxel-treated, Supplementary Figure 4f, g). In addition, animals treated with paclitaxel displayed shorter axons that entered early (n = 42 paclitaxel, n = 16 DMSO, p = 0.0270, Student’s t-test) and larger axonal angles as measured from the point of axon bifurcation to the DRG soma (n = 42 paclitaxel, n = 15 DMSO, p = 0.0004, Student’s t-test) (Supplementary Figure 4j, k). These results are consistent with the hypothesis that paclitaxel-treated axons induce invasive structures and enter the spinal cord prematurely.
We also validated axon entry with a second, complementary approach. Tumor necrosis factor-ɑ (TNFɑ) is upregulated at pioneer axons as they enter the DREZ6. We treated Tg(tnfa:gfp) animals with SU6656, paclitaxel, or DMSO at 36 hpf and quantified the number of Tg(tnfa:gfp)+ DRG at 56 hpf to visualize a temporal gradient of DRG entry. If paclitaxel causes premature entry, then paclitaxel-treated animals should have increased numbers of Tg(tnfa:gfp)+ DRG compared to DMSO-treated animals in posterior DRG. Our results showed that paclitaxel treatment resulted in an average of 15.5 Tg(tnfa:gfp)+ DRG (n = 50 animals), compared to 9.83 in DMSO controls (n = 48 animals) and 1.35 in SU6656-treated animals at 56 hpf (n = 86 animals) (Fig. 5d–f). Consistent with the hypothesis that paclitaxel and SU6656 effect spinal invasion and entry, whole animal profiles of Tg(tnfa:gfp)+ DRG showed a loss of anterior Tg(tnfa:gfp)+ DRG in SU6656-treated animals compared to DMSO. Meanwhile, an expansion of posterior Tg(tnfa:gfp)+ DRG in paclitaxel-treated animals was observed compared to DMSO (Fig. 5f). We ensured that the observed tnfa expression was in the DRG by treating Tg(tnfa:gfp); Tg(sox10:mrfp) with SU6656 or paclitaxel. In both DMSO-treated and paclitaxel-treated animals by 72 hpf, 100% of pioneer neurons express GFP in DMSO-treated compared to 51.7% of SU6656-treated pioneer neurons (n = 60 DMSO-treated, n = 68 paclitaxel-treated, n = 118 SU6656-treated) (Supplementary Figure 4l, m). These results support the hypothesis that precise regulation of invasion components at the DREZ drives axon entry.
Invasion structures in pioneer axons are required for entry
We next tested the hypothesis that actin-rich invasion structures were specifically required in the growth cones of pioneer axons. Rac1 drives disassembly of invadopodia, an invasive structure that mimics our Lifeact-GFP concentrates33. We therefore manipulated Rac1 specifically in pioneer axons using a photoactivable Rac1. We expressed PA-Rac1 in pioneer axons by injecting uas:PA-Rac1-mcherry into Tg(sox10:gal4); Tg(uas:lifeact-gfp). We confirmed the expression of PA-Rac1-mcherry by detecting mCherry+ puncta in pioneer axons (Fig. 6a). Rac1 was photoactivated during DREZ entry and navigation by exposing the tissue to 445 nm light every 5 min for 24 h. As a control, PA-Rac1 expressing neurons were imaged without exposure to 445 nm. In this experiment, 80% of unactivated PA-Rac1 neurons produced Lifeact-GFP concentrates compared to 10% of activated PA-Rac1 neurons (Fig. 6b, c, n = 9 unactivated, n = 10 activated). Similarly, 10% of activated PA-Rac1 axons entered the spinal cord compared to 80% of unactivated controls (Fig. 6d, n = 9 unactivated, n = 10 activated). Activated PA-Rac1 DRG still stall at the DREZ but fail to form stable Lifeact-GFP structures (Fig. 6c, e). Meanwhile, unactivated controls stall and form actin concentrates normally. Together, these data support the hypothesis that invasive structures are cell autonomously required in pioneering growth cones for spinal cord entry.
Invasion components colocalize with invadopodia indicators
Since the actin-rich invasion components in pioneer axons respond to pharmacological treatments and molecular triggers that alter invadopodia, we used immunohistochemistry to test the localization of invadopodia molecules during axon entry. Invadopodia recruit Cortactin and a phosphorylated form of Src to drive their formation9. We stained Tg(sox10:lifeact-gfp) animals at 56 hpf to visualize localization of these components with actin concentrates at the DREZ. Cortactin localized specifically at the growth cone at the DREZ (Fig. 6f). Using deconvolution software we visualized that this punctate pattern of Cortactin colocalized with Lifeact-GFP puncta that were basally projecting (Fig. 6f). pSrc also colocalized to the growth cone at the DREZ (Fig. 6g). Together, these data are consistent with the hypothesis that the invasion components utilized during axon entry are invadopodia9,10,34.
Invadopodia defects can be rescued with spinal lesions
Our data thus far indicate that actin-based invasion is dynamically employed to breach the glia limitans. This implies that pioneer axons could enter the spinal cord despite invadopodia inhibition if a coherent glia limitans is absent. To test this we asked if DREZ lesioning could rescue axon entry in SU6656-treated animals. We did this by treating Tg(sox10:lifeact-GFP); Tg(gfap:nsfb-mcherry) animals with SU6656 or DMSO at 36 hpf, lesioning the DREZ at 48 hpf, and then scored navigation and invadopodia formation in pioneer axons from 48 to 72 hpf (Fig. 7a, Supplementary Movie 8). In SU6656-treated animals with lesioned DREZ the Lifeact-GFP peak was shorter, consistent with SU6656 treatment (Supplementary Figure 5a-d). We confirmed the lesion by measuring a difference in the Tg(gfap:nsfb-mcherry) intensity in lesioned and non-lesioned DREZ (Supplementary Figure 5e). In SU6656-treated non-lesioned DREZ, pioneer axons rarely entered the spinal cord. However, SU6656-treated animals with lesioned DREZ fully recovered spinal cord entry (Fig. 7b). These data are consistent with the hypothesis that invadopodia are dispensable for pioneer axon entry when an intact DREZ is absent.
We next used a complementary approach of Tg(tnfa:gfp) expression to test the above hypothesis. To test this we treated Tg(tnfa:gfp); Tg(gfap:nsfb-mcherry) animals with SU6656 or DMSO at 36 hpf, lesioned the DREZ at 48 hpf, and then scored Tg(tnfa:gfp) expression in pioneer axons at 72 hpf. In SU6656-treated animals with lesioned DREZ, 65% of DRG neurons expressed Tg(tnfa:gfp), a rescue from SU6656-treated non-lesioned DREZ (Fig. 7c). Based on these collective data, we propose that invadopodia induce axon entry into the spinal cord and crossing of the glia limitans in the absence of boundary cap cells (Fig. 7d).
Somatosensory nerve development requires the coordination of neuronal and glial cells. Using time-lapse imaging we first demonstrate that boundary cap cells are not present at the DREZ during pioneer axon entry, altering our understanding of how DRG axons traverse at the nascent DREZ. Instead, invadopodia dynamically form in a distinct growth cone structure when pioneer axons approach the DREZ and are essential for axons to breach the spinal cord glia limitans. Using laser-induced lesions of spinal tissue we show that failed invadopodia formation and axon entry can be rescued by creating an artificial breach of the glia limitans at the DREZ. Together, the simplest explanation for these combined data is that pioneer axons employ a unique growth cone structure at minimum composed of invadopodia to cross the spinal cord boundary.
Boundary cap cells are neural crest-derived cells that reside at both the DREZ and motor exit point7,35,36,37. Some reports have observed that axons preferentially cross into the spinal cord at the sites of boundary cap cells, leading to the hypothesis that boundary cap cells guide DRG axon ingrowth7. Based on the collective data we propose, the invasion and boundary cap ingrowth hypotheses are both likely but separated temporally in development: pioneer axons utilize invadopodia to enter and secondary axons enter via neural crest cells that reside at or near the DREZ7.
Axon navigation through space utilizes distinct and dynamic growth cone morphologies8,10,38,39,40,41. In addition to the classical growth cone structures of filopodia and lamellipodia, invadopodia have recently been added to the repertoire of growth cone machineries10. Specifically, invadopodia are required during early motor axon navigation, providing a potential link between axon guidance studies and invasion through packed tissues. We identify a precise time in development where a growth cone switches morphology within ~100 min: filopodia before entry, to invadopodia during entry, and back to filopodia following entry. Our data suggest that the DREZ could serve as a model to study the interaction between guidance cues and growth cone morphologies, linking two well-studied fields: axon guidance and cell invasion.
Axonal invadopodia colocalize with Cortactin and pSrc. Further, we modulate the invasive capacity of pioneer axons by inhibiting Src family kinases. We also identified Rac1 as a negative regulator of invasion components in DRG pioneer axons. Together, these results are consistent with reports of invadopodia formation in other contexts, including growth cones in vitro9,10,27,42,43,44. Invadopodia are essential in at least three distinct neurodevelopmental times: neural crest migration27, motor axon navigation10, and pioneer axon entry. Evidence suggesting the reuse of these components is particularly intriguing since defects could disrupt multiple stages of circuit formation.
Contact for reagent and resource sharing
Further information and requests for resources and reagents should be directed to the Lead Contact, Cody J. Smith (firstname.lastname@example.org).
Experimental model and subject details
All animal studies were approved by and complied with the University of Notre Dame Institutional Animal Care and Use Committee. Stable zebrafish strains used for this study were as follows: AB, Tg(ngn1:gfp)12, Tg(sox10:mrfp)19, Tg(gfap:gfp)20, Tg(sox10:gal4)15, Tg(uas:lifeact-gfp)24, Tg(gfap:nsfb-mcherry)25, Tg(tnfa:gfp)45, and Tg(sox10:eos)17, Tg(uas:mcherry)16. A transgenic Tg(sox10:mrfp); ngn1:egfp-caax was generated by injecting a ngn1:egfp-caax construct into Tg(sox10:mrfp) embryos at a 75 ng/µl concentration and Tol2 396 transposase messenger RNA (mRNA). F0 embryos were imaged for mosaic analysis. This construct was made using the −3.1 kb ngn1 promoter46.
Embryos were produced from pairwise matings and raised at 28 °C in egg water in constant darkness and staged by hours or days post fertilization47. Embryos of either sex were used for all experiments.
In vivo imaging
Embryos were manually dechorionated at 48 hpf and anesthetized with 3-amino-benzoic acid ester (Tricaine). Anesthetized embryos were immersed in 0.8% low-melting point agarose and mounted on their right side in glass-bottomed 35 mm Petri dishes48. A spinning disk confocal microscope from 3i technology© was utilized and is equipped with a Zeiss Axio Observer Z1 Advanced Mariana Microscope with X-cite 120LED White Light LED System and filter cubes for GFP and mRFP, a motorized X,Y stage, piezo Z stage, 20X Air (0.50 NA) objective with 2 mm working distance, 63× (1.15 NA) water objective with 0.66 mm working distance, 40× (1.1 NA) water objective with 0.62 mm working distance, CSU-W1 T2 Spinning Disk Confocal Head (50 μM) with 1× camera adapter, and/or iXon3 1Kx1K EMCCD camera, dichroic mirrors for 446, 515, 561, 405, 488, 561, 640 excitation, laser stack containing 405 nm, 445 nm, 488 nm, 561 nm, and 637 nm with laser stack FiberSwitcher that has 250 μs switch time, photomanipulation with vector© high speed point scanner ablations at diffraction limited capacity, Ablate!TM© Photoablation System (532 nm pulsed laser, pulse energy 60J @ 200 HZ). All images of DRG were taken in the trunk of the animal. Time lapse images were taken every 5 min for 24 h starting at 48 hpf. Adobe Illustrator and ImageJ were used to process images and enhance image brightness and contrast.
Radial glia focal lesions
Focal lesions of the radial glia membrane were created using the Ablate!TM© Photoablation System described above. Two lesions of 10–12 µm were created approximately 10 µm from the bottom of the radial glial membrane (the location of the DREZ) in each animal at 48 hpf. Adjacent nerves with non-lesioned DREZ areas were used as controls. After focal lesioning, time-lapse images of the nerves were taken as described above.
The primary antibodies used in this study were Zrf-1 (1:100, mouse, ZIRC, ZFIN ID: ZDB-ATB-081002–46), anti-Sox10 (1:5000, rabbit, Kucenas lab)49, anti-Cortactin (1:200, mouse, Sigma, catalog number: SAB4500766)10, and anti-pSrc (Y418) (1:200, rabbit, Invitrogen, catalog number: 44–660G)10. The secondary antibodies used were Alexa Flour 594 goat anti-rabbit (1:600, Invitrogen, catalog number: A-11037), Alexa Flour 594 goat anti-mouse (1:600, Invitrogen, catalog number: R37121), and Alexa Fluor 647 goat anti-mouse (1:600, Invitrogen, catalog number: A-21235). Larvae were fixed using 4% paraformaldehyde in PBST (phosphate-buffered saline (PBS) with 0.1% Triton X-100) at room temperature (25 °C) for 3 h. The fixed larvae were washed with PBST, deionized water with 1% Triton X-100, and acetone for 5 min each, and incubated in acetone at −30 °C for 15 min. Larvae were washed 3 times with PBST for 5 min and incubated with 5% goat serum in PBST for 1 h at room temperature. The larvae were then incubated with the primary antibody solution for 1 h at room temperature and then transferred to 4 °C overnight. After 3 washes with PBST for 30 min and a wash with PBST for 1 h, the larvae were incubated with the secondary antibody solution for 1 h at room temperature and then transferred to 4 °C overnight. After 3 washes in PBST for 1 h, larvae were stored in 50% glycerol in PBS at 4 °C until imaging. Larvae were mounted and still images were taken using the same protocol as previously described for in vivo imaging.
The chemical reagents used for this study were SU6656 (Santa Cruz Biotechnology), paclitaxel (Acros), GM6001 (Santa Cruz Biotechnology), purvalanol A (Tocris), and U0126 (Cayman). Stock solutions of these reagents were kept at −20 °C with concentrations of 375 µM (SU6656), 2.2 mM (paclitaxel), and 1.0 mM (GM6001, purvalanol A and U0126) in DMSO. Treated embryos were dechorionated at 36 hpf and incubated with 3 µM (SU6656)27, 22 µM (paclitaxel)50, and 10 µM (GM6001, purvalanol A and U0126) in egg water until imaging28. Control animals were incubated with 1% DMSO in egg water.
Intravital zebrafish imaging
Tg(tnfa:gfp) animals were incubated with SU6656, paclitaxel, or DMSO and imaged using a Zeiss Axiozoom microscope equipped with 4 filter cubes (4′,6-diamidino-2-phenylindole (DAPI), GFP, RFP, and 641 nm) and a monochrome camera run by Zen software at 56 hpf. The number of Tg(tnfa:gfp)+ DRG were scored for each treatment. Images were taken with a monochrome camera run by Zen software. Images were processed using Adobe Photoshop to adjust brightness and contrast.
Creation of the psELN07 (ngn1:megfp:pa+cmcl2:gfp) DNA construct was generated using the Gateway LR Clonease II Plus system (ThermoFisher) using zebrafish compatible Tol2 vectors51. A p5e-ngn1(−3.1 kb) vector was used to drive expression in sensory neurons using the 3.1 kb upstream promotor region for the ngn1 gene46. For expression of membrane-tethered eGFP, we used the pMe-eGFP−CAAX and p3e-PA. Multiple site gateway recombination of these vectors was accomplished using linearized pDestTol2CG2.
A tol2–4xnr UAS-PA Rac1-mcherry plasmid was diluted to a working solution of 75 ng/µl. This working solution was further diluted to 12 ng/µl in water along with 25 ng/µl of transposase mRNA. This injection solution was injected into single-cell Tg(sox10:gal4); Tg(uas:lifeact-GFP) embryos. At 48 h, injected embryos were screened for mcherry expression via confocal microscopy. mcherry+ DRG were imaged for 24 h either with or without exposure to 445 nm light. Mature PA-Rac1 photoactivates upon exposure to 445 nm light. tol2–4xnr UAS-PA Rac1-mcherry was a gift from Anna Huttenlocher (Addgene plasmid #41878).
Tracing of growth cones
ImageJ plugin MTrackJ was used for tracking individual growth cones. Movies were converted to Tiff-OME and each time point within a 24-h movie was manually tracked. Individual scientists who performed the tracking were blind to the hypothesis and predicted outcome of the given experiment. Accuracy of the tracks was verified by a second scientist.
Axon entry measurements
Y-orthogonal images of the glia limitans and navigating axons were generated by digitally rotating images 90° using Slidebook software. These images were converted to Tiff-OME files and the y- and z-planes of the image were traced in ImageJ. For the quantifications, the y-plane was established as the edge of the glia limitans, and the z-plane was horizontal plane of the y-orthogonal image through the growth cone as determined by the Tg(sox10:lifeact-GFP) signal. From these tracings, the intensities of the Tg(gfap:nsfb-mcherry) and Tg(sox10:lifeact-GFP) signals were individually plotted over the distance of the tracing of the plane by the plot profile analysis in ImageJ.
Quantification and statistical analysis
Slidebook software was used to generate composite z-images for the cell and nerve counts. Individual z-images were sequentially observed to confirm composite accuracy. All graphically presented data unless otherwise noted represent the mean of the analyzed data. Growth cone tracking was performed using the MTrackJ plugin for ImageJ, and all distances were collected using this software. Intensity values were collected with the MTrackJ plugin for ImageJ and normalized using the background intensity. The period before entry was defined as the 20 time points preceding the growth cone’s approach to the DREZ, the period of entry was defined as the 20 time points following the growth cone’s approach to the DREZ, and the period after entry was defined as the next 20 time points. For each of these measurements, the DREZ was defined as the location at which the pioneer axon entered or would enter the spinal cord. An axon was considered to have entered the spinal cord if its axon bifurcated after approaching the DREZ. Independent verification of this entry was then completed by rotating the images 90 degrees to visualize a cross-section. GraphPad Prism software was used to determine statistical analysis. Supplementary Table 1 represents the statistical parameters used in all figure panels.
Further information on experimental design is available in the Nature Research Reporting Summary linked to this article.
All data generated in this manuscript are present in the figures and supplemental figures.
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We thank Marc Wolman, Crislyn D’Souza-Schorey, Bernard Kulemaka, David Hyde, and members of the Smith lab for their helpful comments and reagent guidance, Sam Connell and Brent Redford of 3i for fielding imaging questions, and Deborah Bang, Karen Heed, and Kay Stewart for zebrafish care. This work was supported by the University of Notre Dame, the Elizabeth and Michael Gallagher Family, the Alfred P. Sloan Foundation, Center for Zebrafish Research at the University of Notre, and Center of Stem Cells and Regenerative Medicine at the University of Notre Dame.
The authors declare no competing interests.
Journal peer review information: Nature Communications thanks Pate Skene and the other anonymous reviewer(s) for their contribution to the peer review of this work.
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Nichols, E.L., Smith, C.J. Pioneer axons employ Cajal’s battering ram to enter the spinal cord. Nat Commun 10, 562 (2019). https://doi.org/10.1038/s41467-019-08421-9
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