1. Developmental Biology
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Spinal cord precursors utilize neural crest cell mechanisms to generate hybrid peripheral myelinating glia

  1. Laura Fontenas
  2. Sarah Kucenas  Is a corresponding author
  1. Department of Biology, University of Virginia, United States
https://doi.org/10.7554/eLife.64267
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  1. Laura Fontenas
  2. Sarah Kucenas
(2021)
Spinal cord precursors utilize neural crest cell mechanisms to generate hybrid peripheral myelinating glia
eLife 10:e64267.
https://doi.org/10.7554/eLife.64267
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Abstract

During development, oligodendrocytes and Schwann cells myelinate central and peripheral nervous system axons, respectively, while motor exit point (MEP) glia are neural tube-derived, peripheral glia that myelinate axonal territory between these populations at MEP transition zones. From which specific neural tube precursors MEP glia are specified, and how they exit the neural tube to migrate onto peripheral motor axons, remain largely unknown. Here, using zebrafish, we found that MEP glia arise from lateral floor plate precursors and require foxd3 to delaminate and exit the spinal cord. Additionally, we show that similar to Schwann cells, MEP glial development depends on axonally derived neuregulin1. Finally, our data demonstrate that overexpressing axonal cues is sufficient to generate additional MEP glia in the spinal cord. Overall, these studies provide new insight into how a novel population of hybrid, peripheral myelinating glia are generated from neural tube precursors and migrate into the periphery.

Introduction

The central and peripheral nervous systems (CNS and PNS, respectively) are two distinct yet connected compartments characterized by molecularly distinct cellular components that communicate to allow information to travel from the CNS to the periphery, and vice versa. Spinal motor nerves, which are composed of motor axons and their associated ensheathing glia, are essential to relay action potentials from the spinal cord to peripheral targets such as muscle. Motor exit point (MEP) transition zones (TZ) are specialized structures where motor axons exit the CNS, and where centrally and peripherally derived myelinating glia meet to myelinate the same axons (Fontenas and Kucenas, 2018; Fraher, 1992; Fraher, 2002). Until recently, TZs were thought to be selectively permeable to only axons, and the establishment of the territories occupied by glial cells remained poorly described and not well understood. Recent work now demonstrates that MEP TZs are occupied by dynamic glial cells and are precisely regulated over the course of nervous system development (Coulpier et al., 2010; Fontenas et al., 2019; Kucenas et al., 2008b; Kucenas et al., 2009; Smith et al., 2016; Smith et al., 2014; Zhu et al., 2019). CNS components such as oligodendrocyte (OL) lineage cells, motor neurons, and radial glia segregate and function in the spinal cord, whereas Schwann cells segregate and function in the PNS. However, other glial cells such as MEP glia, neural crest cells (NCCs), and perineurial glia, freely cross the MEP TZ as spinal motor nerves are being formed (Kucenas et al., 2008b; Smith et al., 2014; Zhu et al., 2019).

During nervous system development, neural tube precursors generate oligodendrocyte progenitor cells (OPC) that differentiate into OLs and ultimately myelinate axonal segments in the CNS, while Schwann cells originate from the neural crest and myelinate axons in the PNS (Bergles and Richardson, 2015; Jessen and Mirsky, 2005). Recently, we described MEP glia, a population of CNS-derived, peripheral glial cells that originate in the neural tube, exit through the MEP TZ, and eventually reside just outside of the spinal cord along motor nerve root axons, occupying territory between Schwann cells in the periphery and OLs in the spinal cord (Smith et al., 2014). In addition to their central origin and ultimate peripheral fate, one of the unique features of MEP glia is their expression of both CNS and PNS identity markers, including olig2 and foxd3 (Fontenas and Kucenas, 2018; Smith et al., 2014). MEP glia express foxd3 before they exit the neural tube, and its expression persists as they migrate into the periphery along motor axons (Smith et al., 2014). Although the function of foxd3 in maintaining the fate of NCCs and repressing melanogenesis is known in chick, Xenopus, zebrafish, and mouse, its role in the ventral neural tube where MEP glia originate, remains unknown (Dottori et al., 2001; Kos et al., 2001; Lister et al., 2006; Sasai et al., 2001; Teng et al., 2008).

Once in the periphery, MEP glia tightly associate with spinal motor root axons and ultimately myelinate the most proximal axonal segments along the nerve, and therefore, participate in the fast conduction of action potentials from the CNS to the muscle (Fontenas and Kucenas, 2018; Smith et al., 2014). Previously, we showed that MEP glia also function to restrict highly migratory OPCs to the spinal cord (Fontenas et al., 2019; Smith et al., 2014). While we are beginning to appreciate the functional roles of MEP glia (Fontenas et al., 2019; Smith et al., 2014), we still lack a complete understanding of their development. MEP glia originate within the ventral neural tube, however, their precise origin and relationship to other CNS cell populations and peripheral Schwann cells, remain unclear (Smith et al., 2014).

Here, we describe the mechanisms that control MEP glial development. Using a combination of live imaging, clonal analysis, and genetic approaches in zebrafish, we show that MEP glia originate from nkx2.2a+/olig2+ radial glial precursors and require foxd3 to delaminate from the lateral floor plate and exit the spinal cord via MEP TZs. We also show that MEP glia require axonal cues and classical NCC signaling cascades to migrate out of the spinal cord. We demonstrate that similar to Schwann cells, MEP glial development is driven by axonal Neuregulin signaling and that manipulating this signaling is sufficient to generate additional MEP glia from precursors in the post-embryonic spinal cord. Together, our results demonstrate that ventral spinal cord precursors employ NCC developmental mechanisms to generate hybrid, peripheral myelinating glia and bring a better understanding of MEP glial development and spinal motor nerve formation.

Results

Nkx2.2a+/olig2+/foxd3+ neural tube radial glial precursors give rise to MEP glia

Although all peripheral myelinating glia were previously thought to originate from the neural crest, we recently described MEP glia, a population of peripheral spinal motor nerve root glia that are derived from olig2+ ventral spinal cord precursors and exit the CNS to myelinate peripheral motor axons (Figure 1A; Smith et al., 2014). In our initial study, we reported that MEP glia originate from olig2+ precursors in the spinal cord and like perineurial glia, exit the CNS through MEP TZs at approximately 48 hr post-fertilization (hpf). However, the precise mechanisms that govern their development remained uninvestigated (Kucenas et al., 2008b; Smith et al., 2014).

Figure 1 with 3 supplements see all
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MEP glia are hybrid, centrally derived, peripheral myelinating glia.

(A) Timeline of MEP glial development. MEP glia (purple) are specified in the ventral spinal cord (gray) after 36 hpf, exit through motor exit points at ~50 hpf, divide, and migrate to eventually initiate myelination of motor root axons (pink) starting at 72 hpf. mn: motorneuron, LFP: lateral floor plate. (B–F) Lateral views of the motor exit point showing (B) a nkx2.2a+/foxd3+ MEP glia (outlined arrowhead) exiting the spinal cord at the motor exit point at 48 hr post-fertilization (hpf); (C) an olig2+/foxd3+ MEP glia (outlined arrowhead) along motor nerve root axons at 55 hpf; (D) sox10+/nkx2.2a+ MEP glia (outlined arrowheads) and sox10-/nkx2.2a+ perineurial glia (arrow) at 72 hpf; (E) sox10+/nkx2.2a+ MEP glial sheaths (outlined arrowheads) and sox10-/nkx2.2a+ perineurial cells at 4 days post-fertilization dp (arrowhead) and (F) foxd3+ MEP glia making mbp+ myelin sheaths (outlined arrowheads) at 4 dpf. Insets show single z-plane images. (G) In olig2:egfp and nkx2.2a:nls-egfp larvae at 55 hpf, olig2+ pMN domain cells (teal), OPCs (gray), and MEP glia (purple) are labeled, as are nkx2.2a+ LFP cells (yellow), OPCs (gray) and MEP glia (purple). These images were used for fluorescence intensity measurement. (H) Violin plot of mean intensity of GFP fluorescence of olig2:egfp+ cells at 55 hpf (OPCs: 54914 ± 1674 arbitrary units (A.U.), MEP glia: 7149 ± 394, pMN domain cells: 29934 ± 1481). (I) Violin plot of mean intensity of GFP fluorescence of nkx2.2a:nls- egfp cells at 55 hpf (OPCs: 22981 ± 2013, MEP glia: 28610 ± 1624, lateral floor plate cells: 24049 ± 1602). (H–I) (n = 28 MEP glia, n = 28 OPCs and n = 28 neural tube cells from seven embryos). Asterisks denote the dorsal root ganglion (DRG) and yellow dashed lines denote the edge of the spinal cord. Scale bar (B–G) 20 µm.

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The vertebrate embryo neural tube is organized according to the expression of region-specific transcription factors along the antero-posterior and dorso-ventral axis in a spatially and temporally controlled manner. Precursor cells produce different cell types in a stereotypical sequence and the fate of the progeny is determined by when and where they were born (Briscoe et al., 2000). For example, distinct olig2-expressing neural precursors in the pMN domain sequentially generate motor neurons and oligodendrocytes (Fu et al., 2002; Ravanelli and Appel, 2015; Zhou et al., 2001). Nkx2.2a precursors, which lie just ventral to the pMN domain, generate interneurons, OLs, and perineurial glia, a subpopulation of centrally-derived peripheral glia that form the perineurium along motor nerves (Briscoe et al., 1999; Clark et al., 2014; Deska-Gauthier et al., 2020; Fu et al., 2002; Kucenas et al., 2008a; Kucenas et al., 2008b; Morris et al., 2017; Schäfer et al., 2007; Soula et al., 2001).

To investigate the origin of MEP glia and characterize their molecular identity in the periphery, we used in vivo imaging in different combinations of zebrafish transgenic lines between 48 hpf and 4 days post-fertilization (dpf). To visualize and distinguish MEP glia from perineurial glia, we used the foxd3:mcherry gene trap line, where foxd3 regulatory sequences label NCCs and MEP glia (Fontenas and Kucenas, 2018; Hochgreb-Hägele and Bronner, 2013; Smith et al., 2014), in combination with the ventral spinal cord reporter lines nkx2.2a:nls-egfp and nkx2.2a:mcerulean, where nkx2.2a regulatory sequences label the p3 domain (lateral floor plate) of the ventral spinal cord and its derivatives, including perineurial glia (Zhu et al., 2019). We began our imaging at 48 hpf as this is when we first observe CNS-derived, peripheral glia exiting the neural tube. At 48 hpf in nkx2.2a:nls-egfp;foxd3:mcherry embryos, we observed that MEP glia express the lateral floor plate marker nkx2.2a (Figure 1B and Figure 1—figure supplement 1A), which we and others had not previously observed, while perineurial glia, which also exit the spinal cord at approximately 50 hpf, expressed only nkx2.2a (Figure 1B and Figure 1—figure supplement 1A,B; Kucenas et al., 2008b). From these observations, we conclude that nkx2.2a is a new marker for MEP glia.

To confirm that the CNS-derived nkx2.2a+/foxd3+ cells we observed and the olig2+/foxd3+ MEP glia that we previously described were the same cells, we imaged foxd3:mcherry;olig2:egfp embryos, where olig2 regulatory sequences label motor neurons, oligodendrocyte lineage cells, and MEP glia (Fontenas and Kucenas, 2018; Park et al., 2007; Smith et al., 2014). Consistent with previous studies, we found that MEP glia transiently expressed olig2 until approximately 55 hpf (Figure 1C and Figure 1—figure supplement 1C; Fontenas and Kucenas, 2018; Lee et al., 2020; Smith et al., 2014). In all of our live imaging from 48 hpf to 4 dpf, MEP glia were the only nkx2.2a+/foxd3+ or olig2+/foxd3+ cells we detected in both the CNS and the PNS.

We next sought to verify that the foxd3+/nkx2.2a+ motor nerve-associated glia that we observed were MEP glia and not perineurial glia (Kucenas et al., 2008b). To do this, we used the sox10:tagrfp transgenic line, where sox10 regulatory sequences label glia, including MEP glia, Schwann cells, and OLs, but not perineurial glia (Binari et al., 2013; Kucenas et al., 2008b; Zhu et al., 2019). At 72 hpf in nkx2.2a:nls-egfp;sox10:tagrfp larvae, we observed both nkx2.2a+/sox10+ MEP glia and nkx2.2a+/sox10- perineurial glia along motor nerve axons (Figure 1D). When we looked at 4 dpf in nkx2.2a:megfp;sox10:mrfp larvae, we observed two morphologically distinct cell types, with nkx2.2a+/sox10+ MEP glial membrane sheaths that were reminiscent of myelin internodes (Almeida et al., 2011; Almeida et al., 2018; Fontenas and Kucenas, 2018; Preston et al., 2019), and nkx2.2a+/sox10- loose perineurial cell membranes (Figure 1E; Binari et al., 2013; Kucenas et al., 2008b). To confirm that these nkx2.2a+/sox10+ sheaths along motor root axons were the same MEP glial myelin sheaths that we described previously (Smith et al., 2014), we imaged foxd3:mcherry;mbp:egfp-caax larvae, where mbpa regulatory sequences drive expression of membrane-tethered eGFP in myelinating glia (Almeida et al., 2011). At 4 dpf, we observed mbp+ myelin sheaths formed by foxd3+ cells along motor root axons just outside of the spinal cord (Figure 1F), in a pattern consistent with the location and morphology of MEP glia. By examining various combinations of double transgenic embryos and larvae, we conclude that MEP glia are foxd3+/sox10+/olig2+/nkx2.2a+/mbp+ neural-tube-derived, peripheral myelinating glia that express a unique combination of central and peripheral markers, and identify nkx2.2a as a new marker for MEP glia.

In our imaging, we detected olig2 expression in MEP glia. However, GFP fluorescence dramatically diminished shortly after they exited from the spinal cord (Figure 1C). Quantification of the eGFP fluorescence intensity in 55 hpf olig2:egfp embryos showed that MEP glial levels of eGFP were 4.18 times lower than olig2+ cells of the pMN domain and 7.68 times lower than OPCs (Figure 1G,H). Additionally, in situ hybridization with a mRNA probe specific to olig2 did not show olig2+ cell bodies in the PNS near the MEP TZ at 48 or 72 hpf (Figure 1—figure supplement 1D), demonstrating that MEP glia turn off olig2 before they exit the CNS. However, measurements of the eGFP fluorescence intensity in 55 hpf nkx2.2a:nls-egfp embryos revealed no statistically significant difference in expression between MEP glia, lateral floor plate cells, and OPCs (Figure 1G,I). To confirm these findings, we also measured GFP fluorescence levels over the course of MEP glial development in the CNS and PNS using foxd3:mcherry;nkx2.2a:nls-egfp and foxd3:mcherry;olig2:egfp embryos and larvae at 48, 50, 55, and 72 hpf (Figure 1—figure supplement 2A–C). We observed that while nkx2.2a-driven fluorescence of GFP remained stable after MEP glial exit from the spinal cord (Figure 1—figure supplement 2A,C), we observed a 2.5 fold-decrease in olig2-driven expression of GFP at these same stages (Figure 1—figure supplement 2B,C). Because MEP glia express low levels of olig2 (Figure 1C,G,H) but high levels of nkx2.2a (Figure 1B,D,G,I), and because olig2 and nkx2.2a are identity markers of distinct neural tube precursor domains, we hypothesized that MEP glia originate from the nkx2.2a lateral floor plate and not from the pMN domain as we initially described (Smith et al., 2014).

We therefore investigated the structure of ventral neural tube domains prior to and during MEP glial development. We imaged transverse sections of the developing neural tube in olig2:egfp;nkx2.2a:nls-mcherry embryos and larvae from 24 to 72 hpf, a time window that encompasses the specification and migration of MEP glia. We observed that the olig2 pMN domain and the nkx2.2a lateral floor plate of the neural tube, which are distinct at 24 hpf, lose their defined separation at approximately 30 hpf and merge to give rise to one mixed domain by 48 hpf, a phenomenon that has previously been observed and described during OPC specification (Figure 1—figure supplement 3; Kessaris et al., 2001; Kucenas et al., 2008a; Scott et al., 2020; Soula et al., 2001; Tsai et al., 2020; Xiong et al., 2013). Because MEP glia appear to express both olig2 and nkx2.2a, we hypothesized that similar to OPCs, MEP glia originate from a mixed domain.

To determine if MEP glia come from nkx2.2a+/olig2+ precursors, we analyzed the co-expression of foxd3 with olig2 and nkx2.2a in the ventral spinal cord in foxd3:mcherry;olig2:egfp and foxd3:mcherry;nkx2.2a:mcerulean embryos prior to MEP glial exit. At 48 hpf, we observed foxd3+ MEP glia with weak expression of olig2, just ventral to the pMN domain (Figure 2A). In foxd3:mcherry;nkx2.2a:mcerulean embryos, we observed floor plate foxd3+/nkx2.2a+ MEP glia at 48 hpf (Figure 2B). In all of our imaging, we always detected one foxd3+ cell in the ventral spinal cord per hemi-segment of the zebrafish trunk (Figure 1B, Figure 2A,B, Figure 2—figure supplement 1). Therefore, we hypothesized that the olig2+/foxd3+ MEP glia and the nkx2.2a+/foxd3+ MEP glia were the same cell. To confirm this, we examined single z-planes of transverse sections of the neural tube in foxd3:mcherry;nkx2.2a:mcerulean;olig2:egfp embryos at 48 hpf. Consistent with our hypothesis, we observed olig2+/nkx2.2a+/foxd3+ MEP glia within the mixed olig2/nkx2.2a domain of the spinal cord at 48 hpf (Figure 2C). We also observed that the shape and the position of these cells next to the central canal of the spinal cord were reminiscent of radial glia (Figure 2A–C).

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Ventral neural tube radial glial precursors give rise to MEP glia.

(A) Transverse section of a foxd3:mcherry;olig2:egfp embryo at 48 hpf showing a foxd3+/olig2+ MEP glial cell (outlined arrowhead) ventral to the olig2 pMN domain in the spinal cord. (B) Transverse section of a foxd3:mcherry;nkx2.2a:mcerulean embryo at 48 hpf showing a foxd3+/nkx2.2a+ MEP glial cell (outlined arrowhead). (C) Transverse section of a foxd3:mcherry;nkx2.2a:mcerulean;olig2:egfp embryo at 48 hpf showing a foxd3+/nkx2.2a+/olig2+ triple positive MEP glial cell (outlined arrowhead) in the p3 domain of the neural tube, just ventral to the pMN domain. (D) Transverse section of a nkx2.2a:nls-egfp embryo showing nkx2.2a+/GFAP+ radial glia (outlined arrowhead) at 48 hpf (top panel) and 72 hpf (bottom panel). Yellow dashed lines outline the edge of the spinal cord. Top right corner white boxes show higher magnification of bottom white boxes. Scale bar, (A–D) 10 µm.

Development of the CNS requires supporting and instructive scaffold cells, and this function is widely attributed to radial glia (Hartfuss et al., 2001; McDermott et al., 2005). In the spinal cord, radial glia are the first glial cells distinguishable from the neuroepithelium. They can be identified morphologically by their long radial fibers extending toward the pial surface and their cell bodies located along the ventricular zone, as well as their expression of region-specific transcription factors (Lyons et al., 2003; Ogawa et al., 2005). In addition to their scaffolding role, radial glia also function as neural precursors in the CNS (Fogarty et al., 2005; Johnson et al., 2016; Park et al., 2007). To better visualize the cellular architecture of the developing spinal cord, we labeled radial glia using the Zrf1 antibody which detects Glial Fibrillary Acidic Protein (GFAP) (Trevarrow et al., 1990). We found that all ventral spinal cord nkx2.2a+ cells that we examined were GFAP+ (Figure 2D; Park and Appel, 2003). For this reason, we will refer to MEP glial progenitors as nkx2.2a+ radial glial precursors (Kim et al., 2008a; Kim et al., 2008b). From these studies, we conclude that MEP glia are generated from lateral floor plate nkx2.2a+/olig2+ radial glial precursors, and maintain expression of both CNS and PNS markers once in the PNS.

Foxd3 is essential for MEP glial delamination and exit from the spinal cord

The fact that MEP glia originate from mixed, ventral spinal cord precursors wasn’t surprising to us, given that olig2 and nkx2.2a are expressed by CNS glia (Kucenas et al., 2008a; Park et al., 2007; Soula et al., 2001; Sun et al., 2001; Tatsumi et al., 2018; Zhou et al., 2001). However, while there are many studies describing the roles of foxd3 in peripheral tissue development, none have described a role for this gene in CNS glial development. To elucidate the role of foxd3 in MEP glial development, we used the foxd3:mcherry gene trap zebrafish line, that when bred to homozygosity, creates a foxd3 mutant (Hochgreb-Hägele and Bronner, 2013). While foxd3:mcherry heterozygous larvae label foxd3+ MEP glia as well as neural crest-derived cells, including dorsal root ganglia (DRG) and Schwann cells (Figure 1B–C, Figure 2A–C, Figure 1—figure supplement 1A and Figure 3A), foxd3:mcherry homozygous larvae, which we will refer to as foxd3-/- larvae, lack these neural crest derivatives as well as MEP glia along spinal motor nerve axons (Figure 3A). When we time-lapse imaged olig2:egfp;foxd3:mcherry;foxd3+/- and -/- larvae from 48 to 72 hpf, we observed that foxd3+ MEP glia migrated onto peripheral motor nerves in foxd3+/- siblings (Figure 3A and Video 1), while they stayed in the ventral spinal cord and failed to exit into the periphery in mutants (Figure 3A and Video 2). Because spinal cord OPCs developed at the expected developmental stage (Figure 3A and Video 2) and the morphology and body length of foxd3-/- larvae were comparable to their control siblings (Figure 3B), we ruled out the possibility that failure of MEP glial exit from the spinal cord was the consequence of developmental delay or perturbed neural tube patterning in foxd3-/- larvae. By 72 hpf, foxd3+/- siblings had peripheral MEP glia on 100% of their spinal motor nerve roots (Figure 3A,C). In contrast, we did not observe any MEP glia in the PNS of foxd3-/- larvae (Figure 3A,C). However, we did observe ectopic, peripheral OPCs along motor nerves in foxd3-/- larvae (Figure 3A,D), which is consistent with the absence of peripheral MEP glia (Fontenas et al., 2019; Smith et al., 2014).

Figure 3 with 2 supplements see all
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MEP glia require foxd3 to exit the spinal cord.

(A) MEP TZ in a foxd3:mcherry;olig2:egfp larvae showing foxd3+ MEP glia (white outlined arrowhead) along the motor root of a foxd3+/- control larva and stalled in the spinal cord of a foxd3-/- larva (white arrowhead) at 3 dpf. Note the presence of peripheral OPCs (yellow outlined arrowheads) along motor nerve axons in a foxd3-/- sibling lacking peripheral MEP glia. (B) Bright-field images of foxd3+/- and foxd3-/- siblings at 3 dpf reveal no developmental delay in foxd3-/- larvae. (C) Percentage of motor nerves with MEP glia in foxd3+/- (n = 150 nerves from 10 larvae) and foxd3-/- siblings (n = 270 nerves from 27 larvae) at 3 dpf. (D) Mean ± SEM of peripheral OPCs in olig2:egfp;foxd3:mcherry;foxd3+/- (0.07 ± 0.07, n = 15 larvae) and foxd3-/- (14.07 ± 1.2, n = 27 larvae) larvae at 3 dpf; p<0.0001. (E) Transverse sections of the spinal cord in foxd3:mcherry;foxd3+/- and foxd3-/- larvae showing MEP glia (outlined arrowheads) at the motor nerve root in a control sibling and MEP glia (arrowheads) in the lateral floor plate in a foxd3 mutant at 72 hpf. (F) Immunohistochemistry showing Sox10+/foxd3+ MEP glia (white outlined arrowheads) along motor nerve root axons in a foxd3+/- control embryo, and a Sox10+/foxd3+ MEP glial cell (white arrowhead) stalled in the spinal cord of a foxd3-/- larvae at 3 dpf. Yellow outlined arrowheads show OPCs in the spinal cord in a control larva and along peripheral axons in a foxd3-/- larva. Asterisks denote the DRG in control larvae. Note the absence of DRG in foxd3 mutants. (G) Dot plot of markers first detected in MEP glia, in percent. (H) Control and foxd3 mRNA-injected nkx2.2a:nls-egfp;foxd3:mcherry embryos showing a nkx2.2a+/foxd3+ MEP glia (outlined arrowhead) in the PNS in a control embryo and nkx2.2a+/foxd3+ MEP glia both in the CNS (arrowhead) and PNS (outlined arrowhead) in the injected embryo, at 50 hpf. (I), Mean ± SEM of additional CNS-located MEP glia indicates 0.08 ± 0.03 MEP glia in control embryos (n = 76 hemi-segments from 10 embryos), and 0.54 ± 0.07 MEP glia in foxd3 mRNA injected embryos (n = 78 hemi-segments from 10 embryos) at 50 hpf; p<0.0001. Asterisks denote the DRG and yellow dashed lines denote the edge of the spinal cord. Scale bar, (A, F) 25 µm, (B) 0.5 mm, (E) 10 µm, and (H) 20 µm.

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Video 1
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foxd3+ MEP glia (arrow) exit the spinal cord and migrate onto olig2+ motor axons in foxd3:mcherry;olig2:egfp;foxd3+/- larvae between 48 and 72 hpf.

Images were taken every 15 min and the movie runs at 10 frames per second (fps).

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foxd3+ MEP glia are stalled in the spinal cord (arrow) in foxd3:mcherry;olig2:egfp;foxd3-/- larvae imaged between 48 and 72 hpf.

Images were taken every 15 min and the movie runs at 10 fps.

One possible reason why we failed to observe MEP glia exit the spinal cord in foxd3-/- larvae is due to a failure of differentiation. To test this hypothesis, we performed in situ hybridization for the MEP glial marker wif1 at 3 dpf (Smith et al., 2014). In foxd3 heterozygous larvae, we observed wif1+ MEP glia in the periphery (Figure 3—figure supplement 1A). In contrast, we detected the presence of wif1+ MEP glia at the edge of the spinal cord near the MEP TZ, but not along the motor root, in foxd3-/- larvae (Figure 3—figure supplement 1A). Therefore, we conclude that MEP glia are present and can differentiate in the absence of Foxd3. To rule out the possibility that the foxd3+ cells that we observed in the ventral spinal cord of foxd3-/- larvae were neurons, we performed immunohistochemistry with an anti-HuC antibody, which labels neurons, in foxd3:mcherry;olig2:egfp larvae at 72 hpf. Analysis of single z-plane confocal images revealed that the olig2+/foxd3+ cells we observed in the CNS of foxd3-/- larvae were HuC-, and therefore, not neurons (Figure 3—figure supplement 1B).

Because sox10 is essential for Schwann cell and OL specification and development (Britsch et al., 2001; Dutton et al., 2001; Kuhlbrodt et al., 1998; Takada et al., 2010) and is also expressed by MEP glia, we sought to determine whether MEP glia turn on Sox10 in foxd3-/- larvae. To do this, we performed immunostaining in olig2:egfp;foxd3:mcherry larvae using an antibody specific to zebrafish Sox10 (Binari et al., 2013). We found that similar to MEP glia in the periphery of control larvae, centrally located MEP glia in foxd3-/- larvae were Sox10+ at 72 hpf (Figure 3F). To determine when Sox10 is turned on in MEP glia in relation to foxd3, we analyzed the expression of both markers in foxd3:mcherry;sox10:nls-eos embryos between 36 and 55 hpf. We tracked foxd3+/sox10+ MEP glia as early as we could detect them in the neural tube (between 44 and 48 hpf) by playing our time-lapse movies backwards and investigated which marker they expressed first. From our data, we observed that foxd3 was detected first in 66.66% of the cells we examined, while sox10 expression was detected first in 8.33% of the cells (Figure 3G). In 25% of the cells we analyzed, foxd3 and sox10 were detected simultaneously, likely because we did not detect the cells early enough in their development. From this data, we conclude that sox10 expression in MEP glia is subsequent to, but independent of, foxd3 expression. Taken together, we conclude that MEP glia are specified in foxd3-/- larvae.

To better understand the position of the stalled MEP glial cell in the CNS along the latero-medial axis, we imaged transverse sections of the spinal cord in foxd3:mcherry;foxd3+/- and mutant larvae at 72 hpf (Figure 3E). We found that while MEP glia were present along peripheral motor axons in heterozygous siblings, they were located in the floor plate in foxd3-/- larvae and had a morphology reminiscent of radial glia (Figure 3E). We conclude from these observations that MEP glia do not delaminate from the lateral floor plate in foxd3 mutants.

To begin to elucidate how foxd3 mediates MEP glial exit from the spinal cord, we investigated the role that this transcription factor plays in the development of the neural crest. Electroporation experiments in chick show that ectopic overexpression of foxd3 in the neural tube leads to the delamination of supernumerary neural crest like-cells (Dottori et al., 2001). Therefore, we hypothesized that loss of foxd3 may lead to a failure of delamination of MEP glia from the precursor domain and overexpression would promote it. To test this hypothesis, we injected foxd3 mRNA into one-cell stage nkx2.2a:nls-egfp;foxd3:mcherry embryos. At 55 hpf, we observed supernumerary nkx2.2+/foxd3+ MEP glia-like cells in the CNS of injected embryos (Figure 3H,I). When we time-lapse imaged these larvae from 50 to 72 hpf, we observed that while a single MEP glial cell exited the control spinal cord (Video 3), a supernumerary MEP glial-like cell generated in the lateral floor plate of foxd3 mRNA-injected larvae eventually exited the spinal cord at MEP TZs (Video 4). From these experiments, we conclude that MEP glia delaminate from the lateral floor plate of the spinal cord in a foxd3-dependent manner, analogous to neural crest cell foxd3-dependent delamination and migration (Figure 3—figure supplement 2).

Video 3
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A single nkx2.2a+/foxd3+ MEP glia (arrow) has exited the spinal cord and divides in the PNS in control foxd3:mcherry;nkx2.2a:megfp;nkx2.2a:nls-egfp embryos.

Video on the right is the merge of GFP and mCherry channels. Images were taken every 15 min from 48 to 72 hpf and the movie runs at 10 fps.

Because foxd3 is a transcription factor, we sought to elucidate the downstream molecular mechanisms underlying MEP glial delamination and migration (Cheung et al., 2005; Dottori et al., 2001; Hanna et al., 2002; Kos et al., 2001; Pohl and Knöchel, 2001). The boundary between the CNS and PNS is composed of radial glial endfeet that secrete extracellular matrix components to establish a basal lamina (Fraher et al., 2007; Lee and Song, 2013; Smith et al., 2016). Cells, including neurons and their growth cones, secrete enzymes such as matrix metalloproteinases (MMPs) to degrade proteins of the extracellular matrix in order to migrate through it (Hehr et al., 2005; McFarlane, 2003; Yong et al., 2001). Therefore, we hypothesized that MEP glial exit from the CNS requires extracellular matrix degradation. To test this hypothesis, we inhibited MMPs prior to MEP glial exit. We treated nkx2.2a:megfp;foxd3:mcherry embryos with either 100 μM of the global MMP inhibitor GM6001 in 1% DMSO, or 1% DMSO alone, from 36 hpf on and time-lapse imaged MEP glial migration at TZs from 45 to 55 hpf and from 55 hpf to 72 hpf. At 48 hpf, we observed nkx2.2a+/foxd3+ MEP glia delaminate from the lateral floor plate and exit the spinal cord in DMSO-treated control larvae (Figure 4A and Video 5). In contrast, in GM6001-treated larvae, we detected delamination of nkx2.2a+/foxd3+ MEP glia from the lateral floor plate, but they stalled at the edge of the CNS/PNS boundary and rarely exited into the periphery (Figure 4A and Video 6). To determine if MEP glial exit was delayed under these conditions, we quantified the number of MEP glia present in the spinal cord or along motor nerves at 55 and 72 hpf (Figure 4B,C). Quantification revealed that while 90.61% MEP glia exited the spinal cord in control larvae by 55 hpf, only 8.58% migrated out of the spinal cord when MMPs were inhibited, and 53.01% were stalled in the CNS (Figure 4B). By 72 hpf, 100% of MEP glia were found in the PNS of control larvae, whereas 46.65% were located in the spinal cord of GM6001-treated larvae and only 31.78% were present along spinal motor nerves (Figure 4C). To visualize the location of the stalled MEP glia, we imaged transverse sections of control or drug-treated foxd3:mcherry;nkx2.2a:megfp larvae and observed foxd3+/nkx2.2a+ MEP glia in the PNS of DMSO-treated larvae (Figure 4D). In contrast, we often observed foxd3+/nkx2.2a+ MEP glia stalled in the CNS of GM6001-treated larvae at 72 hpf, in a position adjacent to the midline (Figure 4D). From these results, we conclude that blocking MMPs inhibits MEP glial migration out of the spinal cord and phenocopies the foxd3 mutant phenotype.

Figure 4
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Matrix metalloproteinases participate in MEP glial exit.

(A) Lateral view of the zebrafish trunk showing a nkx2.2a+/foxd3+ MEP glial cell (outlined arrowhead) delaminate from the lateral floor plate and exit the spinal cord in a control embryo and nkx2.2a+/foxd3+ MEP glia unable to exit the spinal cord (white arrowhead) in an embryo treated with 100 µM GM6001 from 36 to 48 hpf. (B) Percentage of MEP glia in the spinal cord, absent, or present along motor nerves at 55 hpf in DMSO control (n = 68 nerves from six embryos) and GM6001- treated embryos (n = 68 nerves from eight embryos). (C) Percentage of MEP glia in the spinal cord, absent, or present along motor nerves at 72 hpf in DMSO control (n = 70 nerves from seven larvae) and GM6001-treated larvae (n = 70 nerves from seven larvae). (D) Transverse sections of foxd3:mcherry;nkx2.2a:megfp spinal cords at 72 hpf showing nkx2.2a+/foxd3+ MEP glia in the PNS (outlined arrowheads) in DMSO control and nkx2.2a+/foxd3+ MEP glia in the lateral floor plate (arrowhead) in GM6001-treated larvae. Yellow dashed lines outline the edge of the spinal cord. (E) In situ hybridizations showing mmp17b in the spinal cord of foxd3+/- and foxd3-/- siblings and adamts3 expression in the spinal cord of foxd3+/- and foxd3-/- siblings and foxd3 mRNA injected embryos at 48 hpf. Scale bar, (A, D, E) 10 µm.

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An additional nkx2.2a+/foxd3+ MEP glia (arrow) exits the spinal cord in foxd3 mRNA-injected foxd3:mcherry;nkx2.2a:megfp;nkx2.2a:nls-egfp embryos.

Video on the right is the merge of GFP and mCherry channels. Images were taken every 15 min from 50 to 72 hpf and the movie runs at 10 fps.

Video 5
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One foxd3+/nkx2.2a+ MEP glial progenitor delaminates from the lateral floor plate, exits the spinal cord, and divides to give rise to several MEP glia along the motor nerve in a foxd3:mcherry;nkx2.2a:megfp control embryo.

Images were taken every 10 min from 48 to 72 hpf and the movie runs at 10 fps.

Video 6
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One foxd3+/nkx2.2a+ MEP glial progenitor delaminates from the lateral floor plate and stalls at the MEP in the spinal cord in a foxd3:mcherry;nkx2.2a:megfp embryo treated with GM6001 from 36 to 72 hpf.

Images were taken every 10 min from 48 to 72 hpf and the movie runs at 10 fps.

Global inhibition of MMPs phenocopied the MEP glial phenotype we observed in foxd3-/- larvae and this led us to hypothesize that foxd3 controls MEP glial exit through the regulation of MMP expression. MMPs are known to play a role in NCC migration in zebrafish and chick (Andrieu et al., 2020; Leigh et al., 2013). Therefore, we asked whether expression of MMPs was perturbed in the ventral neural tube of foxd3 mutant embryos. We investigated the expression of the matrix metalloproteinases mmp17b and adamts3 in WT embryos by in situ hybridization because they have previously been described as involved in NCC migration or were expressed in the embryonic nervous system in the vicinity of MEP TZs (Andrieu et al., 2020; Asakawa et al., 2013; Leigh et al., 2013). From these studies, we found that mmp17b and adamts3 were expressed in the ventral neural tube at 48 hpf, prior to MEP glial exit (Figure 4E). We then assayed their expression in foxd3 mutant embryos to determine if expression of these genes changed. In foxd3-/- embryos, we observed that while expression of mmp17b was unchanged in the spinal cord, adamts3 expression was significantly reduced in the ventral neural tube at 48 hpf (Figure 4E). However, we did not observe any change in adamts3 expression in the spinal cord of embryos overexpressing foxd3 (Figure 4E). Reciprocally, overexpression of human adamTS3 mRNA did not result in more MEP glial delamination from the precursor domain (control: mean ± SEM = 1.06 ± 0.056, n = 18 nerves from five embryos; adamts3 mRNA: mean ± SEM = 1 ± 0.00, n = 29 nerves from nine embryos; p=0.38). Together, these experiments demonstrate the role of MMPs in MEP glial exit and identify adamts3 as one possible candidate downstream of foxd3 signaling in this process.

Neural tube precursors generate one MEP glial cell progenitor per hemi-segment

In our foxd3 mutant analysis, we always observed the presence of one MEP glial cell per somite, stalled inside the spinal cord, just medial to the MEP TZ, in a repetitive pattern along the anterior-posterior axis of the neural tube (Figure 3A,E and F). Additionally, our time-lapse movies consistently showed one cell exiting the spinal cord at MEP TZs and dividing in the periphery in control embryos (Video 7). This led us to hypothesize that radial glial precursors give rise to a single MEP glial cell progenitor per hemi-segment. To test this hypothesis, we used Zebrabow (zebrafish Brainbow), a multispectral cell labeling tool developed for cell tracing and lineage analysis (Brockway et al., 2019; Pan et al., 2013). Zebrabow consists of Cre recombinase-driven, random combinatorial expression of three spectrally distinct fluorescent proteins: cyan, red, and yellow (CFP, RFP, and YFP, respectively). The random combination of fluorescent proteins resulting from Cre recombination results in more than 30 colors and provides a way to distinguish adjacent cells for lineage analysis. Colors are inherited equally among daughter cells and remain stable throughout development (Pan et al., 2013). We used the broadly expressed Zebrabow ubi:zebrabow transgenic line that drives RFP expression ubiquitously, and we created a tissue-specific nkx2.2a:cre transgenic line that drives expression of Cre recombinase in nkx2.2a+ cells. As a first step, to make sure we were lineage-tracing MEP glia, as perineurial glia would also be labeled with our nkx2.2a:cre transgenic line (Kucenas et al., 2008b), we performed an immunostaining against Sox10 and examined nkx2.2a+/Sox10+ MEP glia present along motor axons in nkx2.2a:cre;ubi:zebrabow larvae (Figure 5A). When we looked at the color profile of 214 nkx2.2a+/Sox10+ MEP glia along 60 motor nerves at 4 dpf in confocal z-stack images, we found that 96.67% of MEP glia present along a single motor nerve were the same color, and therefore, originated from the same nkx2.2a+ precursor (Figure 5B).

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Clonal analysis reveals that neural tube precursors give rise to one MEP glial progenitor per motor exit point.

(A) Lateral view of Sox10 immunohistochemistry in a nkx2.2a:cre;ubi:zebrabow larvae showing Cre recombinase driven recombination (blue and green) in nkx2.2a+ cells at 4 dpf. Floor plate cells (bracket) and Sox10+ MEP glia along two distinct nerves (white and yellow outlined arrowheads respectively) labeled. (B) Percentage of MEP glia present along a single motor nerve sharing a common (96.67%) vs distinct neural tube precursor (3.33%); n = 214 MEP glia and n = 60 motor nerves in 20 animals. (C) Ternary plot showing the intensity profile of 14 MEP glia present on three adjacent motor nerves (white and yellow symbols in C correspond to white and yellow outlined arrowheads in A) for RFP, YFP and CFP, in percent. (D) Mean ± SEM of MEP glial cell divisions per motor nerve (2.19 ± 0.18) between 48 and 72 hpf; n = 27 nerves in 12 larvae. (E) DMSO control and aphidicolin/hydroxyurea (HUA)-treated nkx2.2a:nls-egfp;foxd3:mcherry larvae showing nkx2.2a+/ foxd3+ MEP glia (outlined arrowheads) along motor nerve root axons at 72 hpf. (F) Mean ± SEM of MEP glia along motor nerve roots at 72 hpf indicating 2.82 ± 0.12 MEP glia in control larvae (n = 79 hemi-segments from 10 larvae), and 0.90 ± 0.04 MEP glia in aphidicolin/HUA treated larvae (n = 89 hemi-segments from 10 larvae; p<0.0001). (G) Lateral view of a foxd3:mcherry;sox2:egfp larvae at 55 hpf showing foxd3+/sox2+ MEP glia (white outlined arrowhead) and DRG (asterisk). (H) Singe z plane transverse section of a BLBP immunostaining in foxd3:mcherry;nkx2.2a:mcerulean larvae showing BLBP+/foxd3+/nkx2.2a+ MEP glia (outlined arrowheads) outside the spinal cord along the motor nerve root at 55 hpf. Asterisks denote the DRG and yellow dashed lines denote the edge of the spinal cord. Scale bar, (A) 25 µm, (E, H) 20 µm, (G) 10 µm.

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One nkx2.2a+/foxd3+ MEP glial progenitor exits the spinal cord at the MEP transition zone and undergoes cell division in the PNS to generate several MEP glia in a nkx2.2a:nls-egfp/foxd3:mcherry embryo.

Images were taken every 15 min from 50 to 72 hpf and the movie runs at 10 fps.

In order to illustrate the relationship between color profile and lineage in our zebrabow paradigm in a more thorough and unbiased way, we analyzed the color profile of 14 individual MEP glia distributed along three adjacent motor nerves by measuring the fluorescence intensity in the RFP, YFP, and CFP channels separately and plotted the percentage of red, green (YFP was acquired in the green channel), and blue fluorescence (Figure 5C). Using a ternary plot, we observed that the color profiles of MEP glia that were present along the same motor nerve always clustered together (yellow dots cluster together, pink dots cluster together, and white dots cluster together), while fluorescent profiles of MEP glia present along distinct nerves segregated, indicating that MEP glia along the same nerve share a common progenitor, and that each hemi-segment has a single, unique MEP glial progenitor (Figure 5C).

To confirm that MEP glia populate motor nerves by undergoing cell division, we assessed MEP glial proliferation shortly after they exited the spinal cord. To do this, we treated nkx2.2a:nls-egfp embryos with EdU (5-ethynyl-2’-deoxyuridine) from 50 to 56 hpf, in order to detect DNA synthesis in proliferative cells (Figure 5—figure supplement 1A). To quantify proliferative MEP glia, we did an immunostaining against Sox10 and counted the percentage of nkx2.2a+/Sox10+/EdU+ cells in the PNS at 72 hpf (Figure 5—figure supplement 1B–C). We found that 74% of the MEP glia we imaged at 72 hpf were EdU+ and therefore, proliferated between 50 and 56 hpf. We also quantified MEP glial cell division in our time-lapse movies between 48 and 72 hpf and observed 1 to 4 MEP glial cell divisions along motor nerve axons (Figure 5D), which generated up to six cells per nerve by 4 dpf (Figure 5—figure supplement 1D). From these studies we conclude that MEP glia populate motor nerve roots by undergoing cell division.

As an independent approach to investigating whether a single CNS-derived MEP glial cell divides several times to give rise to all the MEP glia located on a single motor nerve, we blocked cell proliferation just as MEP glia exit the spinal cord. To do this, we treated nkx2.2a:nls-egfp;foxd3:mcherry embryos at 44 hpf with a combination of 150 μm aphidicolin and 20 mM hydroxyurea (HUA) in order to arrest the cell cycle at approximately 48 hpf (Lyons et al., 2005). A previous study has demonstrated that just 4 hr of exposure to this cocktail robustly inhibits proliferation of glia in zebrafish (Lyons et al., 2005). When we imaged larvae at 72 hpf, we detected several MEP glia per motor nerve in DMSO-treated larvae, but only saw one MEP glial cell per hemi-segment along motor nerve roots in aphidicolin and HUA-treated larvae (Figure 5E,F and Figure 5—figure supplement 1D). This data supports our hypothesis that CNS precursors give rise to a single MEP glial progenitor cell per hemi-segment in the neural tube, and that this cell exits the CNS and acts as a progenitor that further divides to give rise to all MEP glia found on a single motor nerve.

To test whether MEP glia have other progenitor characteristics, we created a sox2:egfp transgenic line where sox2 regulatory sequences drive eGFP in neural progenitors. We imaged sox2:egfp;foxd3:mcherry embryos and larvae and detected foxd3+/sox2+ MEP glia in the PNS at 52 hpf (Figure 5G) and as late as 5 dpf (Figure 5—figure supplement 1E), revealing that some MEP glia maintain a progenitor state. In light of these observations, we performed an immunostaining directed against another neural progenitor marker, brain lipid binding protein (BLBP), also known as fatty acid binding protein 7 (fabp7), in nkx2.2a:mcerulean;foxd3:mcherry larvae at 55 hpf. In these larvae, we observed BLBP+/nkx2.2a+/foxd3+ MEP glia along motor nerve root axons at 55 hpf (Figure 5H). Together, these results show that MEP glia along the same nerve come from a single progenitor and divide several times to populate spinal motor nerve root axons.

MEP glial development requires axonal cues

Once in the periphery, MEP glia migrate along spinal motor root axons. Because they reside along the same axons as Schwann cells, and because interactions with axons are essential for Schwann cell migration, development, and function (Fontenas et al., 2016; Gilmour et al., 2002; Lyons et al., 2005; Miyamoto et al., 2017; Perlin et al., 2011; Voas et al., 2007), we hypothesized that MEP glial development also depends on axonal cues. To examine whether axonal cues are sufficient to attract MEP glia from the spinal cord to the PNS, we first took advantage of plexinA3 mutants, also known as sidetracked, which lack the semaphorin receptor plexinA3 (Palaisa and Granato, 2007). PlexinA3 mutants are characterized by intraspinal motor axon guidance defects that result in ectopic, supernumerary MEP TZs where motor axons ectopically exit into the periphery. We hypothesized that if axons were sufficient to attract MEP glia out of the spinal cord, plexinA3-/- ectopic motor axons would be associated with MEP glia. We used sox10:eos;nbt:dsred embryos, where nbt regulatory sequences label all neurons and axons (Peri and Nüsslein-Volhard, 2008). We then used UV light-induced photoconversion of sox10:eos embryos at 48 hpf to distinguish between red, photoconverted neural crest-derived Schwann cells from green, non-photoconverted MEP glia and OL lineage cells, as previously described (Smith et al., 2014). We then imaged photoconverted plexina3;nbt:dsred;sox10:eos mutant and WT siblings from 48 to 72 hpf and observed the presence of MEP glia along every motor nerve, including ectopic ones, in both mutant and WT larvae (Figure 6A and Figure 6—figure supplement 1A–B). From this data, we conclude that motor axons are sufficient to induce MEP glial migration into the periphery.

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MEP glial development is axonal dependent.

(A) Lateral view of sox10:eos;nbt:dsred WT control and plexinA3-/- siblings at 3 dpf showing MEP glia along both motor nerve axons (outlined arrowheads) and ectopic motor nerve axons (arrowheads). Brackets denote ectopic motor exit points. (B) Lateral views of sox10:tagrfp;hb9:yfp-ntr larvae from 48 to 72 hpf, treated with either 2% DMSO or 20 mM metronidazole(MTZ)/2% DMSO from 9 to 72 hpf, showing sox10+ MEP glia (white outlined arrowheads) exit the spinal cord and migrate onto healthy motor axons in the control embryo. In the MTZ-treated larvae, MEP glia did not exit the spinal cord. Asterisks denote the DRG and yellow dashed lines denote the edge of the spinal cord. Scale bar, (A) 25 µm, (B) 20 µm.

In order to confirm the role of motor axons in MEP glial migration, we sought to examine if motor axons were required for MEP glial development. To do this, we used sox10:tagrfp;hb9:yfp-ntr embryos, where hb9 regulatory sequences drive expression of YFP and the bacterial enzyme nitroreductase in motor neurons (Mathias et al., 2014; Zhu et al., 2019). Nitroreductase converts the prodrug metronidazole (MTZ) into a cytotoxic drug and allows for temporally controlled, targeted-cell ablation (Curado et al., 2008). We treated hb9:yfp-ntr;sox10:tagrfp embryos with 20 mM MTZ in 2% DMSO starting from 9 hpf, prior to motor neuron specification, and assessed the presence of MEP glia in the periphery using in vivo, time-lapse imaging between 48 and 72 hpf. In these studies, we did not detect any MEP glial migration out of the spinal cord at MEP TZs where motor nerves were genetically ablated (Figure 6B). In these time-lapse movies, OPCs in the spinal cord and Schwann cells along sensory nerves both developed and migrated normally. To ensure that the absence of MEP glia in the PNS was not due to a specification failure, we examined expression of wif1 at the conclusion of our time-lapse acquisition. At 72 hpf, we detected wif1+ MEP glia along motor roots in control larvae (Figure 6—figure supplement 2A). In contrast, we only observed wif1 expression inside the spinal cord of MTZ-treated hb9:yfp-ntr larvae (Figure 6—figure supplement 2A). To better visualize MEP glia in the spinal cord of motor neuron ablated embryos, we treated hb9:yfp-ntr;foxd3:mcherry embryos with MTZ and looked at foxd3+ MEP glia between 50 and 72 hpf. While we saw foxd3+ peripheral MEP glia along motor axons in control larvae, we only saw spinal cord-located foxd3+ MEP glia in MTZ-treated larvae at both 50 and 72 hpf and did not see any along degenerating motor axons (Figure 6—figure supplement 2B). We conclude from these experiments that spinal motor axons are necessary and sufficient to drive MEP glial migration into the PNS.

Neuregulin 1 type III drives MEP glial migration

Numerous studies demonstrate that axonally-derived Neuregulin1 type III is essential for many aspects of Schwann cell development, including directed migration, proliferation, and myelination along motor axons (Heermann and Schwab, 2013; Lee et al., 2020; Lyons et al., 2005; Meyer et al., 1997; Miyamoto et al., 2017; Newbern and Birchmeier, 2010; Perlin et al., 2011; Taveggia et al., 2005). We previously observed that MEP glia are absent along spinal motor nerves in erbb3b mutants and erbb3b is expressed all along the motor nerve including at motor roots (Langworthy and Appel, 2012; Smith et al., 2014). Therefore, we chose to examine the role of neuregulin 1 type III (nrg1) in MEP glial migration. We first investigated the presence of MEP glia in nrg1 zebrafish mutants (Perlin et al., 2011) by using photoconversion to differentially label MEP glia and Schwann cells and live imaging in sox10:eos embryos (McGraw et al., 2012). In nrg1+/+;sox10:eos larvae, we observed red, photoconverted DRG and Schwann cells, and green, non-photoconverted MEP glia along spinal motor nerve root axons (Figure 7A). In contrast, in nrg1-/-;sox10:eos larvae, MEP glia and Schwann cells were absent from motor nerve roots at 72 hpf (Figure 7A), consistent with a recent study showing a reduction in sox10+ cell numbers along motor nerves in nrg1 morpholino-mediated knockdown zebrafish larvae (Lee et al., 2020). Consistent with other previous work, we also did not detect the presence of neural-crest-derived DRG in nrg1 mutants (Honjo et al., 2008). We did, however, observe the presence of sox10+ processes projecting through the MEP TZ along motor nerve root axons in nrg1-/-;sox10:eos larvae (Figure 7A). To identify the origin of these processes, we segmented the confocal images to identify individual cells and pseudo-colored in white the cell that was the closest to the MEP TZ (Figure 7A). By analyzing its morphology, we observed that in WT larvae, the cell that is the most proximal to the MEP TZ is a MEP glial cell, located in the PNS (Figure 7A). In nrg1 mutant larvae, the only cell that is present at the MEP TZ is located in the CNS, has the morphology of an OPC, and projects a process through the MEP (Figure 7A). To confirm that the projections we observed from within the CNS were OPC processes, we did an in situ hybridization for the oligodendrocyte myelin marker proteolipid protein 1a (plp1a), that is not expressed by peripheral myelinating glia in zebrafish (Brösamle and Halpern, 2002; Kucenas et al., 2009; Smith et al., 2014). We observed that while plp1a was expressed in the white matter of the spinal cord in WT larvae, it was also found in the PNS in nrg1-/- larvae (Figure 7—figure supplement 1A).

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Neuregulin 1 type III drives MEP glial directed migration.

(A) Motor exit point of sox10:eos WT and nrg1 -/- siblings photoconverted at 48 hpf and imaged at 3 dpf showing the presence of MEP glia (outlined arrowheads) and Schwann cells (SCs) (arrowhead) in a control larva and the presence of an oligodendrocyte membrane extension (pink arrowhead) in a nrg1 -/- larva that lacks MEP glia and SCs. Yellow dashed lines denote the edge of the spinal cord. (B) In situ hybridization showing wif1+ MEP glia along motor nerve root axons in a WT control larva (outlined arrowheads, n = 24 larvae) and the absence of wif1+ MEP glia along motor nerve root axons in a nrg1 mutant larva at 3 dpf (n = 16 larvae). Arrowheads indicate the presence of wif1+ cells near the lateral line nerve in a nrg1 mutant larva at 3 dpf. (C) In situ hybridization showing wif1+ MEP glia along motor nerve root axons in a WT control larva (outlined arrowheads, n = 20 larvae) and the absence of wif1+ MEP glia along motor nerve root axons in an erbb3b mutant larva at 3 dpf (n = 14 larvae). Arrowheads indicate the presence of wif1+ cells near the lateral line nerve in an erbb3b mutant larva at 3 dpf. Scale bar (A–C), 10 μm.

We then confirmed the absence of MEP glia in nrg1-/- larvae by performing an in situ hybridization for wif1 at 3 dpf and observed wif1+ MEP glia at the MEP TZ in WT larvae (Figure 7B and Figure 7—figure supplement 1B). In contrast, we did not detect any wif1+ MEP glia along spinal motor roots in nrg1-/- larvae (Figure 7B). However, we found wif1+ cells further distally along the motor nerve in the periphery (Figure 7B and Figure 7—figure supplement 1B), that we never observed in WT siblings and consistent with previous work showing wif1+ cells along the lateral line nerve in nrg1 mutants (Lush and Piotrowski, 2014). To confirm that nrg1 functions in MEP glia through erbb3b receptors like in Schwann cells, we also assayed wif1 expression in erbb3b mutants. In 72 hpf erbb3b larvae, wif1+ cells were not exclusively found along motor root axons as in wild-type larvae (Figure 7C), but instead were found more distally in the trunk near the lateral line nerve (Figure 7C), similar to the nrg1 mutant phenotype (Figure 7B and Lush and Piotrowski, 2014). Taken together, we conclude that nrg1 expressed on motor axons drives MEP glial migration to the motor root, and in its absence, MEP glia exit the spinal cord, but fail to associate with motor root axons and migrate away.

To investigate whether axonally derived nrg1 is sufficient to induce MEP glial directed migration, we genetically overexpressed human Neuregulin 1 type III (hNrg1) in most neurons, including spinal cord neurons (Korzh et al., 1998; Liao et al., 1999; Mueller and Wullimann, 2002), using neuroD:gal4;UAS:hNrg1 embryos, where neuroD1 regulatory sequences drive expression of the transcription factor Gal4 (Fontenas et al., 2019) and UAS enhancer sequences drive expression of human Neuregulin 1 type III (Perlin et al., 2011). In these embryos, we detected krox20+ Schwann cells in the white matter of the spinal cord (Figure 8—figure supplement 1) as previously described (Perlin et al., 2011). To determine if MEP glial migration was also affected by overexpression of hNrg1, we first performed an in situ hybridization for wif1 to visualize MEP glia at 3 dpf in neuroD:gal4;UAS:hNrg1 larvae. In neuroD:gal4 control larvae, we observed wif1+ MEP glia exclusively in the periphery along motor root axons (Figure 8A). In contrast, we detected wif1+ MEP glia both in the PNS and in the ventral spinal cord in neuroD:gal4;UAS:hNrg1 larvae (Figure 8A). Because our cell lineage studies showed that just one MEP glial cell is specified in the neural tube at each MEP TZ, we sought to determine whether these centrally-located MEP glia migrated into the spinal cord from the PNS, or conversely, if they were ectopically specified CNS MEP glia-like cells. To do this, we used time-lapse imaging in either nkx2.2a:nls-egfp or sox10:nls-eos larvae to visualize MEP glia in the PNS. In both neuroD:gal4;UAS:hNrg1 and neuroD:gal4 control larvae, we never saw any nkx2.2a+ or sox10+ peripheral MEP glia migrate into the spinal cord between 48 and 72 hpf. However, when we imaged nkx2.2a:nls-egfp;foxd3:mcherry larvae, which label MEP glia more specifically, we detected several nkx2.2a+/foxd3+ MEP glia in the ventrolateral spinal cord of neuroD:gal4;UAS:hNrg1;nkx2.2a:nls-egfp;foxd3:mcherry larvae at 3 dpf (Figure 8B,C), something that we rarely observed in neuroD:gal4;nkx2.2a:nls-egfp;foxd3:mcherry control siblings (Figure 8B,C).

Figure 8 with 2 supplements see all
Download asset Open asset
Neuregulin 1 type III drives MEP glial development.

(A) In situ hybridization showing wif1+ MEP glia (white outlined arrowheads) along motor nerve roots in WT larvae (n = 30 larvae) at 3 dpf and both inside (green outlined arrowheads) and outside (white outlined arrowheads) the spinal cord in neuroD:gal4;UAS:hNrg1 larvae (n = 30 larvae). Zrf1 immunostaining shows GFAP+ radial glia and denotes the outline of the spinal cord. (B) Lateral view of 3 dpf nkx2.2a:nls-egfp;foxd3:mcherry control and neuroD:gal4;UAS:hNrg1 larvae showing nkx2.2a+/foxd3+ MEP glia (outlined arrowheads) along motor nerve root axons. MEP glia are found in both the PNS (outlined arrowheads) and in the ventral spinal cord (arrowheads) in neuroD:gal4;UAS:hNrg1 larvae. Asterisks denote the DRG. (C) Mean ± SEM of additional, centrally located MEP glia per hemi-segment in control (0.17 ± 0.11; n = 12 larvae) and neuroD:gal4;UAS:hNrg1 larvae (1.3 ± 0.3; n = 20 larvae) at 3 dpf. (D) PH3 immunostaining on spinal cord transverse sections in neuroD:gal4;nkx2.2a:nls-egfp control larvae and neuroD:gal4;UAS:hNrg1;nkx2.2a:nls-egfp larvae showing PH3+/nkx2.2a+ proliferating radial glia (outline arrowheads). (E) Mean ± SEM of PH3+/nkx2.2a+ cells in the ventral spinal cord per 20 µm section in neuroD:gal4 (0.35 ± 0.12; n = 17 sections from four embryos) and neuroD:gal4;UAS:hNrg1 larvae (1.22 ± 0.3; n = 18 sections from four embryos). (F) Transverse section of a nkx2.2a:megfp larva at 4 dpf showing Sox2+/nkx2.2a+ radial glial precursors. Yellow dashed lines denote the edge of the spinal cord. Scale bar (A,B,D,F), 10 µm.

Figure 8—source data 1

Source data for Figure 8 .

https://cdn.elifesciences.org/articles/64267/elife-64267-fig8-data1-v2.xlsx

Because Schwann cell proliferation is driven by neuregulin/Erbb signaling (Perlin et al., 2011; Taveggia et al., 2005), we hypothesized that these centrally located MEP glia originate from increased neural tube nkx2.2a+ radial glial precursor divisions. To test this hypothesis, we assessed nkx2.2a+ cell proliferation in the neural tube in neuroD:gal4;UAS:hNrg1;nkx2.2a:nls-egfp and neuroD:gal4;nkx2.2a:nls-egfp embryos by immunolabeling Phospho-HistoneH3 (PH3)+ mitotic cells at 48 hpf (Figure 8D,E). Quantification of ventral spinal cord PH3+/nkx2.2a+ cells revealed an increase in proliferation in neuroD:gal4;UAS:hNrg1 larvae compared to their neuroD:gal4 control siblings (Figure 8D,E). To test whether nrg1 also drives MEP glial proliferation along motor nerves, we treated nkx2.2a:nls-egfp embryos with EdU from 50 to 56 hpf and performed a Sox10 immunostaining at 72 hpf to distinguish MEP glia from perineurial glia (Figure 8—figure supplement 2A), as described in Figure 5—figure supplement 1. At 72 hpf, we observed an increase in the number of EdU+/nkx2.2.a+/Sox10+ MEP glia (Figure 8—figure supplement 2B), as well as an increase in the total number of MEP glia present along motor nerves (Figure 8—figure supplement 2C). Together, these results suggest that nrg1 regulates both MEP glial progenitors and MEP glial proliferation.

To confirm that ventral spinal cord nkx2.2a+ radial glia have the potential to generate MEP glia in post-embryonic development, we performed an immunostaining directed against the progenitor marker Sox2 in nkx2.2a:megfp larvae (Figure 8F). At 4 dpf, we detected the presence of Sox2+/nkx2.2a+ radial glial progenitors in WT larvae, which is the latest stage we have assessed (Figure 8F). This suggests that nkx2.2a+ radial glial precursors are still present in the spinal cord in post-embryonic development and neuregulin1 can control their proliferation.

Discussion

During nervous system development, neural progenitors orchestrate the formation of the brain, spinal cord, and peripheral nerves by generating neurons and glia. Although components of the CNS and PNS are traditionally thought to segregate, growing numbers of studies show the selective and bidirectional permeability of nervous system TZs (Clark et al., 2014; Fontenas et al., 2019; Garcia-Diaz et al., 2019; Green et al., 2019; Kucenas et al., 2008b; Smith et al., 2016; Smith et al., 2014; Zhu et al., 2019). Development of myelinating cells such as oligodendrocytes and Schwann cells has extensively been studied, but development of MEP glia, a novel population of CNS-derived, peripheral glia that freely migrate across TZs, remains poorly understood. In this study, we demonstrate that MEP glia originate from nkx2.2a+ lateral floor plate radial glia and use NCC-associated mechanisms to migrate out of the spinal cord onto motor nerves, where they develop with mechanisms similar to that of Schwann cells.

MEP glia originate from lateral floor plate radial glia and require foxd3 to delaminate and exit the neural tube

The origin of the main central and peripheral myelinating glia has been known for decades. Olig2+ pMN precursors give rise to OL lineage cells and NCCs give rise to Schwann cells (Jessen and Mirsky, 1999; Park et al., 2002; Zhou et al., 2001). Our observations reveal that MEP glia originate from nkx2.2a+ lateral floor plate radial glial precursors that lie just ventral to the olig2 pMN domain of the neural tube and identify nkx2.2a as a new marker for MEP glia. Our study depicts a more detailed picture of these hybrid, centrally derived, peripheral glia that express a unique set of both CNS and PNS glial markers, including nkx2.2a, olig2, sox10, foxd3, the boundary cap cell marker wif1, and make mbp+ myelin sheaths along spinal motor nerve root axons (Coulpier et al., 2009; Feng et al., 1994; Hochgreb-Hägele and Bronner, 2013; Johnson et al., 2016; Kucenas et al., 2008a; Montero-Balaguer et al., 2006; Qi et al., 2001; Smith et al., 2014; Soula et al., 2001; Zhou et al., 2001).

Olig2 and nkx2.2a are two well-known identity markers of cells born in the ventral neural tube and their expression by MEP glia was not unexpected (Briscoe et al., 1999; Park, 2004; Park et al., 2002; Qi et al., 2001; Rowitch, 2004; Zhou et al., 2001). However, foxd3 is known as an early neural crest marker and its function in early steps of NCC development is conserved across all vertebrate species (Fairchild et al., 2014; Hochgreb-Hägele and Bronner, 2013; Lister et al., 2006; Montero-Balaguer et al., 2006; Sasai et al., 2001; Teng et al., 2008). Therefore, both its expression and function in neural tube-derived glia are thought-provoking. Studies in various vertebrate species demonstrate that foxd3 is not necessary for neural crest specification, but is required for NCC migration (Fairchild et al., 2014; Lister et al., 2006; Pohl and Knöchel, 2001; Wang et al., 2011). Similarly, our loss-of-function study shows that foxd3 is also not essential for MEP glial specification, but rather, is required for their delamination and exit from the neural tube and that the latter is at least partially controlled by MMPs. Interestingly, electroporation of tagged-Foxd3 in the chick neural tube leads to the delamination of Foxd3+ cells from the neural tube (Dottori et al., 2001). When we tested whether overexpressing foxd3 in zebrafish was sufficient to induce ectopic delamination and/or exit of lateral floor plate cells, we found an increase in the number of MEP glia that delaminate and exit the CNS.

MEP glial development depends on axonal Neuregulin 1 type III

Our time-lapse movies and clonal analysis reveal that nkx2.2a+ radial glia generate one MEP glia per hemi-segment, which delaminates from the nkx2.2a domain and exits the spinal cord through a MEP TZ. Following migration onto peripheral nerves, CNS-derived MEP glia divide and give rise to two to six cells per motor nerve by 4 dpf. We show that MEP glia are proliferative and that blocking the cell cycle when MEP glia exit the CNS results in a unique MEP glia per hemi-segment in the PNS. Consistent with this observation, our confocal imaging shows that MEP glia express BLBP and sox2, two markers of neural progenitors, that are important for self-renewal (Mercurio et al., 2019; Owada et al., 1996; Sharifi et al., 2013).

The signals that instruct MEP glia to delaminate from the ventral neural tube to migrate through MEP TZs and onto peripheral motor axons have never been explored. Our work shows that in addition to foxd3, MEP glia require motor axons to exit the spinal cord and are not found in the PNS in larvae where MEP TZs exist, but motor axons were genetically ablated. Conversely, ectopic motor exit points in the sidetracked mutants are always associated with MEP glia. We identified neuregulin 1 type III (nrg1) as one of the axonal cues that drive MEP glial migration. The axonal ligand nrg1 and its receptor erbb3, expressed in SCs, are largely known to play a major role in Schwann cell myelination but also in their migration (Lyons et al., 2005; Miyamoto et al., 2017; Newbern and Birchmeier, 2010; Perlin et al., 2011). Therefore, we chose to examine the role of nrg1 in MEP glial interaction with motor axons and MEP glial migration. Using time-lapse imaging and in situ hybridization, we observed that in nrg1 and erbb3b mutant larvae, after exiting the spinal cord, MEP glia do not associate with motor root axons but instead, keep migrating ventrally toward neuro-muscular junctions. Our analysis demonstrates that MEP glia use at least one of the traditional mechanisms that drive Schwann cell development in order to migrate onto motor nerves. Previous work showed that the Neuregulin receptor errb3b is expressed at MEPs and that MEP glia are disrupted in erbb3 mutants, as they are not present along motor nerve root axons in these mutants (Langworthy and Appel, 2012; Morris et al., 2017; Smith et al., 2014). Reciprocally, we asked whether overexpressing Neuregulin 1 type III in CNS neurons was sufficient to divert MEP glia to the spinal cord. Surprisingly, we found that unlike Schwann cells (Perlin et al., 2011), Nrg1 overexpression is not sufficient to reroute MEP glial migration from the PNS to the CNS, but instead, results in the specification of additional MEP glia from spinal cord nkx2.2a+ radial glial precursors at post-embryonic stages (see Figure 8C,D). These findings raise an intriguing question: how similar are these post-embryonic CNS-located MEP glia to the CNS-born Schwann cells found in spinal cord demyelinating lesions (Zawadzka et al., 2010)? Future studies will be needed to determine whether Nrg1-induced CNS located MEP glia differentiate and myelinate spinal cord axons under both physiological and demyelinating conditions.

Materials and methods

Key resources table
Reagent type
(species)
or resource		DesignationSource or referenceIdentifiersAdditional information
Strain
(Danio rerio)		AB*ZIRCRRID:ZFIN_ZDB-GENO-960809-7
Genetic reagent
(Danio rerio)		Tg(nkx2.2a(3.5):Cre;
cmlc2:eGFP)uva42		This paper
Genetic reagent
(Danio rerio)		Tg(nkx2.2a(3.5):
mCerulean3)uva41		This paper
Genetic reagent
(Danio rerio)		Tg(nkx2.2a(3.5):nls-eGFP)uva1This paper
Genetic reagent
(Danio rerio)		Tg(mbp:
eGFP-CAAX)ue2		Almeida et al., 2011RRID:ZFIN_ZDB-ALT-120103-2
Genetic reagent
(Danio rerio)		Gt(foxd3:
mcherry)ct110R		Hochgreb-Hägele and Bronner, 2013RRID:ZFIN_ZDB-ALT-130314-2
Genetic reagent
(Danio rerio)		Tg(XlTubb:
DsRed) zf148		Peri and Nüsslein-Volhard, 2008RRID:ZFIN_ZDB-ALT-081027-2
Genetic reagent
(Danio rerio)		Tg(neuroD1:Gal4;
cmlc2:eGFP)uva22		Fontenas et al., 2019RRID:ZFIN_ZDB-ALT-191209-8
Genetic reagent
(Danio rerio)		Tg(nkx2.2a(3.5):
nls-mCherry)uva2		Zhu et al., 2019RRID:ZFIN_ZDB-ALT-200513-2
Genetic reagent
(Danio rerio)		Tg(olig2:eGFP)vu12Shin et al., 2003RRID:ZFIN_ZDB-ALT-041129-8
Genetic reagent
(Danio rerio)		Tg(olig2:
DsRed2)vu19		Shin et al., 2003RRID:ZFIN_ZDB-FISH-150901–8168
Genetic reagent
(Danio rerio)		Tg(sox10(4.9):Eos)w9McGraw et al., 2012RRID:ZFIN_ZDB-ALT-110721-1
Genetic reagent
(Danio rerio)		Tg(sox10(4.9):
nls-Eos)w18		McGraw et al., 2012RRID:ZFIN_ZDB-ALT-110721-2
Genetic reagent
(Danio rerio)		Tg(sox10(4.9):
TagRFP)uva5		Zhu et al., 2019RRID:ZFIN_ZDB-ALT-200513–7
Genetic reagent
(Danio rerio)		Tg(sox10(7.2):
mRFP)vu234		Kucenas et al., 2008bRRID:ZFIN_ZDB-ALT-080321–3
Genetic reagent
(Danio rerio)		Tg(UAS:hNrg1
type III)st85		Perlin et al., 2011RRID:ZFIN_ZDB-ALT-120221–8
Genetic reagent
(Danio rerio)		Tg(ubi:
Zebrabow-M)a131		Pan et al., 2013RRID:ZFIN_ZDB-ALT-130816–2
Genetic reagent
(Danio rerio)		Tg(2xNRSE-2xMnx1-
Mmu.Fos:KalTA4,5xUAS-
ADV.E1b:GAP-YFP-2A-Eco.
NfsBT41Q/
N71S/F124T)lmc008		Mathias et al., 2014RRID:ZFIN_ZDB-ALT-151021–5
Genetic reagent
(Danio rerio)		Tg(sox2(2.9):
eGFP)uva55		This paper
Genetic reagent
(Danio rerio)		neuregulin1z26Perlin et al., 2011RRID:ZFIN_ZDB-ALT-120308–1
Genetic reagent
(Danio rerio)		plexinA3 p13umalPalaisa and Granato, 2007RRID:ZFIN_ZDB-ALT-071126–1
Genetic reagent
(Danio rerio)		erbb3bst48Lyons et al., 2005RRID:ZFIN_ZDB-ALT-050512–6
Recombinant
DNA reagent		p5E-nkx2.2a(−3.5)Pauls et al., 2007N/A
Recombinant
DNA reagent		pME-mcerulean3Zhu et al., 2019N/A
Recombinant
DNA reagent		p5E-sox2(−2.9)This paper
Recombinant
DNA reagent		pME-nls-eGFPKwan et al., 2007N/A
Recombinant
DNA reagent		p3E-polyAKwan et al., 2007N/A
Recombinant
DNA reagent		pDestTol2CG2Kwan et al., 2007N/A
Recombinant
DNA reagent		pME-creThis paper
Recombinant
DNA reagent		Human adamts3Genomics-onlineCat.
#ABIN3996515
Commercial
assay or kit		pENTR 5´-TOPO
cloning kit		InvitrogenCat. #K59120
Commercial
assay or kit		LR clonase II plusInvitrogenCat. #12538–120
Commercial
assay or kit		Click-it EdU Cell
proliferation kit
for imaging.
Alexa Fluor 647 dye		InvitrogenCat. #C11340
Commercial
assay or kit		mMESSAGE mMACHINE
sp6 transcription kit		FisherCat. #AM1340
Chemical
compound, drug		DAPI fluoromount-GSouthern BiotechCat. #0100–20
Chemical
compound, drug		DIG RNA labeling mixRocheCat.
#11277073910
Chemical
compound, drug		metronidazoleSigmaCat#M1547;
CAS#443-48-1		20 mM
Chemical
compound, drug		GM6001Enzo Life SciencesCat.
#BML-EI300-0001;
CAS# 142880-36-2		100 μM
Chemical
compound, drug		aphidicolinSigmaCat. #A0781;
CAS# 38966-21-1		150 μM
Chemical
compound, drug		hydroxyureaSigmaCat. #H8627;
CAS#127-07-1		20 mM
AntibodyMouse anti-GFAPZIRCCat. #Zrf1 ;
RRID:AB_10013806		1 :1000
AntibodyAnti-digoxigenin-AP,
Fab fragments
from sheep		SigmaCat#11093274910;
RRID:AB_514497		1:5000
AntibodyRabbit anti-sox10Binari et al., 2013N/A1 :5000
Antibodychicken anti-GFPAbcamCat. #ab13970;
RRID:AB_300798		1 :500
AntibodyAlexa Fluor 488
goat anti-chicken		ThermoFisherCat. #A-11039;
RRID:AB_2534096		1:1000
AntibodyAlexa Fluor 647
goat anti-rabbit
IgG(H+L)		ThermoFisherCat. #A-21244;
RRID:AB_2535812		1:1000
AntibodyRabbit anti-BLBPSigmaCat. #ABN14;
RRID:AB_10000325		1:1000
AntibodyRabbit anti-PH3MilliporeCat. #06–570;
RRID:AB_310177		1:2000
AntibodyRabbit anti-sox2AbcamCat. #ab97959;
RRID:AB_2341193		1:500
AntibodyAlexa Fluor 647
goat anti-mouse
IgG(H+L)		ThermoFisherCat. #A-21235;
RRID:AB_2535804		1:1000
Sequence-based
reagent		Cre-FThis paperPCR primers5’-ATGTCCAATCTTCTAACCGT-3’
Sequence-based
reagent		Cre-RThis paperPCR primers5’-TTAGTCTCCATCCTCCAGCA-3’
Sequence-based
reagent		Foxd3-FThis paperPCR primers5’-CAGGGATCCATGA
CCCTGTCTGGAGGCA-3’
Sequence-based
reagent		Foxd3-RThis paperPCR primers5’-GAACTCGAGTCATTGA
GAAGGCCATTTCGATA-3’
Sequence-based
reagent		Sox2-FThis paperPCR primers5’-GTGAGTAACTTTT
GGGTGTGCGG-3’
Sequence-based
reagent		Sox2-RThis paperPCR primers5’-TTAAACCGATTTTC
TCGAAAGTCTAC-3’
Sequence-based
reagent		Mmp17b-FThis paperPCR primers5’-GGGAAGTGCTG
TGGATGTTT-3’
Sequence-based
reagent		Mmp17b-RThis paperPCR primers5’-TAATACGACTCACTATAGATG
AAACTCGAGCAGTGTTGG-3’
Sequence-based
reagent		Adamts3-FThis paperPCR primers5’-TCCTGGGGCT
AGACATGTGA-3’
Sequence-based
reagent		Adamts3-RThis paperPCR primers5’-TAATACGACTCACTATAGAGC
GCACAGTACGGATTTGA-3’
SoftwareImageJ/FijiImageJ.nih.govRRID:SCR_003070
SoftwarePrism 9GraphPad softwaresRRID:SCR_002798
SoftwareMetamorphMolecular DevicesRRID:SCR_002368
SoftwareImaris 9.6Oxford InstrumentsRRID:SCR_007370
SoftwareRStudioRStudioRRID:SCR_000432

Zebrafish husbandry

Request a detailed protocol

All animal studies were approved by the University of Virginia Institutional Animal Care and Use Committee. Zebrafish strains used in this study were: AB*, neuregulin1z26 (Perlin et al., 2011), erbb3bst48 (Lyons et al., 2005), plexinA3p13umal (Palaisa and Granato, 2007), Gt(foxd3:mcherry)ct110R (Hochgreb-Hägele and Bronner, 2013), Tg(XlTubb:dsred)zf148 (Peri and Nüsslein-Volhard, 2008), Tg(sox10(4.9):nls-Eos)w18, Tg(sox10(4.9):eos)w9(McGraw et al., 2012), Tg(olig2:dsred2)vu19, Tg(olig2:egfp)vu12 (Shin et al., 2003), Tg(nkx2.2a:megfp)vu17 (Kucenas et al., 2008b), Tg(mbp:egfp-caax)ue2 (Almeida et al., 2011), Tg(neuroD:gal4)uva22 (Fontenas et al., 2019), Tg(sox10(7.2):mrfp)vu234 (Kucenas et al., 2008b), Tg(sox10(4.9):tagrfp)uva5, Tg(nkx2.2a(3.5):nls-mcherry)uva2, Tg(nkx2.2a(3.5):nls-egfp)uva1, Tg(ubi:zebrabow-m)a131 (Pan et al., 2013), Tg(UAS:hNrg1typeIII)st85 (Perlin et al., 2011), Tg(hb9:yfp-ntr)lmc008 (Mathias et al., 2014), Tg(nkx2.2a(3.5):mcerulean3)uva41, Tg(nkx2.2a(3.5):cre)uva42, and Tg(sox2(2.9) :egfp)uva55. Table 1 denotes abbreviations used for each mutant and transgenic line. Embryos were raised at 28.5°C in egg water and staged by hours or days post fertilization (hpf and dpf, respectively). Embryos of either sex were used for all experiments (Kimmel et al., 1995). Phenyl-thiourea (PTU) (0.004%) in egg water was used to reduce pigmentation for imaging. Stable, germline transgenic lines were used in all experiments.

Table 1
Strains and transgenic lines.

Picture description: Cross section of the spinal cord showing Sox2+ neural precursors (magenta), nkx2.2a+ precursors (cyan) and Sox10+ glia (yellow) at 4 days post-fertilization.

Full nameabbreviationReference
Tg(mbp:eGFP-CAAX)ue2mbp:egfp-caaxAlmeida et al., 2011
Gt(foxd3:mcherry)ct110Rfoxd3:mcherryHochgreb-Hägele and Bronner, 2013
Tg(XlTubb:DsRed) zf148nbt:dsredPeri and Nüsslein-Volhard, 2008
Tg(neuroD1:Gal4; cmlc2:eGFP)uva22neuroD:Gal4Fontenas et al., 2019
Tg(nkx2.2a:meGFP)vu17nkx2.2a:megfpKucenas et al., 2008b
Tg(nkx2.2a(3.5):Cre; cmlc2:eGFP)uva42nkx2.2a:creThis paper
Tg(nkx2.2a(3.5):mCerulean3)uva41nkx2.2a:mceruleanThis paper
Tg(nkx2.2a(3.5):nls-eGFP)uva1nkx2.2a:nls-egfpThis paper
Tg(nkx2.2a(3.5):nls-mCherry)uva2nkx2.2a:nls-mcherryZhu et al., 2019
Tg(olig2:eGFP)vu12olig2:egfpShin et al., 2003
Tg(olig2:DsRed2)vu19olig2:dsredShin et al., 2003
Tg(sox10(4.9):Eos)w9sox10:eosMcGraw et al., 2012
Tg(sox10(4.9):nls-Eos)w18sox10:nls-eosMcGraw et al., 2012
Tg(sox10(4.9):TagRFP)uva5sox10:tagrfpZhu et al., 2019
Tg(sox10(7.2):mRFP)vu234sox10:mrfpKucenas et al., 2008b
Tg(UAS:hNrg1 type III)UAS:hNrg1Perlin et al., 2011
Tg(ubi:Zebrabow-M)a131ubi:zebrabowPan et al., 2013
Tg(2xNRSE-2xMnx1-Mmu.Fos:KalTA4,5xUAS-ADV.E1b:GAP-YFP-2A-Eco.NfsBT41Q/N71S/F124T)lmc008hb9:yfp-ntrMathias et al., 2014
Tg(sox2(2.9):eGFP)uva55sox2:egfpThis paper
AB*wildtype
neuregulin1z26nrg1Perlin et al., 2011
plexinA3 p13umal (sidetracked)plexinA3Palaisa and Granato, 2007
erbb3bst48erbb3bLyons et al., 2005

Generation of transgenic lines

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All constructs were generated using the Tol2kit Gateway-based cloning system (Kwan et al., 2007). Vectors used for making the expression constructs were p5E-nkx2.2a(−3.5) (Pauls et al., 2007), pME-mcerulean3 (Zhu et al., 2019), pME-Cre, p5E-sox2(−2.9), as well as pME-nls-eGFP, p3E-polyA, pDestTol2pA2 and pDestTol2CG2 destination vectors (Kwan et al., 2007).

To build pME-Cre, we amplified cre coding sequences from pCS2-Cre.zf1 (Horstick et al., 2015) using the following primers: forward primer, 5’-ATGTCCAATCTTCTAACCGT-3’ and reverse primer, 5’-TTAGTCTCCATCCTCCAGCA-3’. The resulting PCR product was subcloned into pCR8/GW/TOPO (Invitrogen) to generate a pME vector for Gateway cloning. pCS2-Cre.zf1 was a gift from Harold Burgess (Addgene plasmid #61391).

To generate the Tg(sox2:egfp) line, we amplified 2.9 kb of sequence immediately upstream of the sox2 gene (NM_213118) from wild-type genomic DNA using the following primers: forward primer, 5’-GTGAGTAACTTTTGGGTGTGCGG-3’ and reverse primer, 5’-TTAAACCGATTTTCTCGAAAGTCTAC-3’. The resulting PCR fragment was subcloned into pENTR 5´-TOPO (Invitrogen) to generate a p5E entry for Gateway cloning. p5E, pME and p3E-polyA vectors were ligated into destination vectors through LR reactions (Ashton et al., 2012). Final constructs were amplified, verified by restriction digests, and sequenced to confirm the insertions. To generate stable transgenic lines, plasmid DNAs were microinjected at a concentration of 25 ng/μL in combination with 10 ng/μL Tol2 transposase mRNA at the one-cell stage and screened for founders (Kawakami, 2004).

Generation of synthetic mRNA

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For foxd3 overexpression experiments, we amplified foxd3 coding sequences using the following primers (forward primer, 5’-CAGGGATCCATGACCCTGTCTGGAGGCA-3’, reverse primer, 5’-GAACTCGAGTCATTGAGAAGGCCATTTCGATA-3’) and subcloned the PCR fragment into pCS2+ with BamH1 and Xho1. The vector was linearized with Not1 and foxd3 mRNA was transcribed using mMESSAGE mMACHINE sp6 transcription kit (Ambion). For adamts3 overexpression experiments, we linearized the pCR-XL-TOPO vector containing human ADAMTS3 full length cDNA (genomics-online.com ABIN3996515) with BamH1 and human adamts3 mRNA was transcribed using mMESSAGE mMACHINE t7 transcription kit (Ambion).

In vivo imaging

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Embryos were anesthetized with 0.01% 3-aminobenzoic acid ester (Tricaine), immersed in 0.8% low-melting point agarose and mounted in glass-bottomed 35 mm Petri dishes (Electron Microscopy Sciences). After mounting, the Petri dish was filled with egg water containing PTU and Tricaine. A 40X water objective (NA = 1.1) mounted on a motorized Zeiss AxioObserver Z1 microscope equipped with a Quorum WaveFX-XI (Quorum Technologies) or Andor CSU-W1 (Oxford Instruments) spinning disc confocal system was used to capture all images. Images were imported into Metamorph (Molecular devices), Image J or Imaris (Oxford Instruments). Images of foxd3:mcherry embryos were deconvolved using the Image J plugin Iterative Deconvolve 3D to reduce background signal. All images were then imported into Adobe Photoshop. Adjustments were limited to levels, contrast, and cropping.

Sectioning

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Embryos were fixed in 4% paraformaldehyde (PFA) at 4°C overnight. After fixation, embryos were embedded in 1.5% agarose/30% sucrose and frozen in 2-methylbutane chilled by immersion in liquid nitrogen. We collected 20 μm transverse sections on microscope slides using a cryostat microtome. Sections were covered with DAPI fluoromount-G (Southern Biotech). A 40X water objective (NA = 1.1) or a 63X water objective (NA = 1.2) mounted on a motorized Zeiss AxioObserver Z1 microscope equipped with a Quorum WaveFX-XI (Quorum Technologies) or Andor CSU-W1 (Andor Oxford Instruments) spinning disc confocal system was used to capture all images. Images were imported into Image J and Adobe Photoshop. Adjustments were limited to levels, contrast, and cropping.

Eos photoconversion

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For whole-embryo Eos photoconversion, Tg(sox10:eos) embryos were mounted for imaging as described above and then exposed to UV light using a DAPI filter for 1 min with a Zeiss Axiozoom V16 microscope at 48 hpf.

Wholemount immunohistochemistry

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Dechorionated embryos were fixed with 4% PFA overnight at 4°C, washed in PBSTx (1% Triton X-100, 1x PBS) for 5 min, permeabilized in acetone at room temperature for 5 min and at −20°C for 10 min, followed by a 5 min wash with PBSTx. Embryos were then blocked in 5% goat serum/PBSTx for 1 hr, incubated in primary antibody with 5% goat serum/PBSTx for 1 hr at room temperature and overnight at 4°C. Embryos were washed extensively with PBSTx at room temperature and incubated in secondary antibody overnight at 4°C. After antibody incubation, embryos were washed extensively with PBSTx and stored in PBS at 4°C until imaging. The following antibodies were used: rabbit anti-Sox10 (1:5000) (Binari et al., 2013), chicken anti-GFP (1:500; abcam), Alexa Fluor 488 goat anti-chicken (1:1000; ThermoFisher) and Alexa Fluor 647 goat anti-rabbit IgG(H+L) (1:1000; ThermoFisher). Embryos were mounted in glass-bottomed Petri dishes for imaging as described above.

Immunohistochemistry on section

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Embryos were fixed in 4% PFA overnight at 4°C and sectioned as described above. Sections were rehydrated in PBS for 30 min and blocked with 5% goat serum/PBS for 1 hr at room temperature. Primary antibody incubation was done overnight at 4°C. Secondary antibody incubation was done for 2 hr at room temperature. Antibodies used were: chicken anti-GFP (1:500; abcam ab13970), mouse anti-GFAP (1:1000; ZIRC zrf-1), rabbit anti-PH3 (1:2000; Millipore 06–570), rabbit anti-BLBP (1:1000; Millipore ABN14), rabbit anti-Sox2 (1:500; abcam ab97959), Alexa Fluor 647 goat anti-rabbit IgG(H+L) (1:1000), Alexa Fluor 488 goat anti-chicken IgG(H+L) (1:1000), Alexa Fluor 647 goat anti-mouse IgG(H+L) (1:1000).

In situ hybridization

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Larvae were fixed in 4% PFA at 4°C overnight and stored in 100% methanol at −20°C and processed for in situ RNA hybridization as described previously (Hauptmann and Gerster, 2000). Plasmids were linearized with appropriate restriction enzymes and cRNA preparation was carried out using Roche DIG-labeling reagents and RNA polymerases (NEB). We used previously published probes for olig2 (Park et al., 2002), plp1a (Brösamle and Halpern, 2002), krox20 (Monk et al., 2009), and wif1 (Smith et al., 2014). Mmp17b and adamts3 probes were generated using the following primers (mmp17b forward primer, 5’-GGGAAGTGCTGTGGATGTTT-3’, reverse primer, 5’-TAATACGACTCACTATAGATGAAACTCGAGCAGTGTTGG-3’; adamts3 forward primer, 5’-TCCTGGGGCTAGACATGTGA-3’, reverse primer, 5’-TAATACGACTCACTATAGAGCGCACAGTACGGATTTGA-3’) and t7 RNA polymerase. Sectioning was performed as described above and sections were covered with Aqua-poly/mount (Polysciences). Images were obtained using a Zeiss AxioObserver inverted microscope equipped with Zen, using a 40x oil immersion objective. All images were imported into Adobe Photoshop. Adjustments were limited to levels, contrast, and cropping.

Chemical treatments

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For motor neuron ablation, dechorionated hb9:yfp-ntr embryos were treated with 20 mM metronidazole (Sigma)/2% DMSO in egg water from 9 to 24 hpf and 20 mM metronidazole/2% DMSO in PTU egg water from 24 to 72 hpf. Control siblings were treated with 2% DMSO in egg water or PTU egg water according to their stage.

For matrix metalloproteinase inhibition experiments, dechorionated foxd3:mcherry;nkx2.2a:megfp embryos were treated with 100 μM GM6001 (Enzo Life Sciences)/1% DMSO in PTU egg water from 36 to 72 hpf. Fresh drug was replaced prior to imaging at 48 hpf. Control siblings were treated with 1% DMSO in PTU egg water.

For cell cycle arrest experiments, dechorionated foxd3:mcherry;nkx2.2a:nls-egfp embryos were treated with 150 μM aphidicolin (Sigma) and 20 mM hydroxyurea (Sigma)/2% DMSO in PTU egg water from 48 to 72 hpf. Control siblings were treated with 2% DMSO in PTU egg water.

For the EdU incorporation assay, nkx2.2a:nls-egfp embryos were treated with 0.1 mM EdU/1% DMSO from 50 to 56 hpf in PTU egg water at 28.5°C, switched to PTU egg water at 56 hpf and fixed for 1 hr in 4% PFA at 72 hpf. Whole embryos were permeabilized with cold acetone for 7 min at −20°C and stained for EdU using the Click-it EdU Cell Proliferation kit for Imaging with Alexa Fluor 647 dye (ThermoFisher), as detailed in the kit protocol. Click-it reaction was performed for 1 hr at room temperature followed by an immunostaining against Sox10 and GFP as described above.

Genotyping

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Genomic DNA was extracted using HotSHOT (hot sodium hydroxide and tris) (Truett et al., 2000). The primers used for genotyping UAS:hNrg1typeIII, erbb3bst48, nrg1z26 and plexinA3p13umal have previously been published (Lyons et al., 2005; Palaisa and Granato, 2007; Perlin et al., 2011).

Quantification and statistical analysis

Fluorescence intensity measurement

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For MEP glial eGFP fluorescence intensity analysis, we measured the mean gray value of four MEP glia, four oligodendrocytes, or four neural tube cells per image and the mean gray value of four regions of background using Image J, and analyzed seven images from seven embryos per transgenic line. We calculated the corrected cell fluorescence intensity by subtracting the background mean gray value.

For the time course analysis of MEP glia eGFP fluorescence intensity, we measured the mean eGFP gray value of foxd3:mcherry+/olig2:egfp+ and foxd3:mcherry+/nkx2.2a:nls-egfp+ MEP glia at 48, 50, 55, and 72 hpf using single z-planes of confocal images. To avoid photobleaching, different groups of embryos from the same clutch were used for each timepoint assessed. For each measurement, the region of interest was defined using the mCherry channel to better visualize MEP glia and measurements were done using the same coordinates in the corresponding GFP channel. For olig2 and nkx2.2a, the mean gray value measured at 48 hpf was normalized to 1 and all mean gray values from the 50, 55, and 72 hpf timepoints were compared to that value. The number of MEP glia used for this analysis is as follows (olig2, 48 hpf: n = 27, 50 hpf: n = 27, 55 hpf: n = 24, 72 hpf: n = 20; and nkx2.2a, 48 hpf: n = 13, 50 hpf: n = 26, 55 hpf: n = 25, 72 hpf: n = 31).

For Zebrabow intensity profile analysis, we split the image channels and measured the mean gray value of each individual MEP glia in the red channel, green channel, and blue channel, in Image J. Individual MEP glia were identified by their x, y, and z coordinates. Percentages of fluorescence of reach channel was calculated by dividing the mean gray value by the maximum intensity of each image using the plugin Histogram. The zebrabow intensity profile ternary plot was made in R studio with the Ternary package.

Quantification of MEP glia and OPC numbers

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Student t tests and for multiple comparisons, one-way ANOVAs followed by Tukey’s multiple comparison tests, were performed using Prism 8. For violin plots, dotted lines represent quartiles and the central dashed line marks the median. The data in plots and the text are presented as means ± SEM.

Data availability

All data generated or analyzed during this study are included in the manuscript and supporting files.

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Article and author information

Author details

  1. Laura Fontenas

    Department of Biology, University of Virginia, Charlottesville, United States
    Contribution
    Conceptualization, Resources, Data curation, Formal analysis, Validation, Investigation, Visualization, Methodology, Writing - original draft, Project administration, Writing - review and editing
    Competing interests
    No competing interests declared
    ORCID icon "This ORCID iD identifies the author of this article:" 0000-0003-0544-0147

  2. Sarah Kucenas

    Department of Biology, University of Virginia, Charlottesville, United States
    Contribution
    Conceptualization, Supervision, Funding acquisition, Validation, Writing - original draft, Project administration, Writing - review and editing
    For correspondence
    sk4ub@virginia.edu
    Competing interests
    No competing interests declared
    ORCID icon "This ORCID iD identifies the author of this article:" 0000-0002-1950-751X

Funding

NINDS (NS072212)

  • Sarah Kucenas

NINDS (NS107525)

  • Sarah Kucenas

The funders had no role in study design, data collection and interpretation, or the decision to submit the work for publication.

Acknowledgements

We thank Lori Tocke for zebrafish care and members of the Kucenas lab for valuable discussions. We thank Drs. Yunlu Zhu, Eyleen O’Rourke, and Sarah Siegrist for helpful suggestions, and Dr. William Talbot for the Tg(UAS:hNrg1typeIII) line. This work was funded by NIH/National Institute of Neurological Disorders and Stroke (NINDS): NS072212 (SK) and NS107525 (SK).

Ethics

Animal experimentation: All animal studies were approved by the University of Virginia Institutional Animal Care and Use Committee, Protocol #3782.

Version history

  1. Received: October 22, 2020
  2. Accepted: February 5, 2021
  3. Accepted Manuscript published: February 8, 2021 (version 1)
  4. Version of Record published: February 16, 2021 (version 2)

Copyright

© 2021, Fontenas and Kucenas

This article is distributed under the terms of the Creative Commons Attribution License, which permits unrestricted use and redistribution provided that the original author and source are credited.

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  1. Laura Fontenas
  2. Sarah Kucenas
(2021)
Spinal cord precursors utilize neural crest cell mechanisms to generate hybrid peripheral myelinating glia
eLife 10:e64267.
https://doi.org/10.7554/eLife.64267

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