Vascular networks surrounding individual organs are important for their development, maintenance, and function; however, how these networks are assembled remains poorly understood. Here we show that CNS progenitors, referred to as radial glia, modulate vascular patterning around the spinal cord by acting as negative regulators. We found that radial glia ablation in zebrafish embryos leads to excessive sprouting of the trunk vessels around the spinal cord, and exclusively those of venous identity. Mechanistically, we determined that radial glia control this process via the Vegf decoy receptor sFlt1: sflt1 mutants exhibit the venous over-sprouting observed in radial glia-ablated larvae, and sFlt1 overexpression rescues it. Genetic mosaic analyses show that sFlt1 function in trunk endothelial cells can limit their over-sprouting. Together, our findings identify CNS-resident progenitors as critical angiogenic regulators that determine the precise patterning of the vasculature around the spinal cord, providing novel insights into vascular network formation around developing organs.https://doi.org/10.7554/eLife.20253.001
Organ vascularization is a fundamental developmental event that is necessary for the establishment and maintenance of organ function. Previous work on the vascularization of different organs has shown that the process starts with angiogenic sprouting from the surrounding vasculature (Kurz et al., 1996; Hogan et al., 2004; Sakaguchi et al., 2008). For instance, the vascularization of the central nervous system (CNS) begins with angiogenic sprouting into neural tissues from the peri-neural vascular plexus (PNVP), a network that surrounds the CNS (Feeney and Watterson, 1946; Strong, 1964; Kurz et al., 1996; Hogan et al., 2004; Bautch and James, 2009). Similarly, liver vascularization has been shown to initiate by angiogenic sprouting from the vessels that first surround it (Sakaguchi et al., 2008). Although different organs undergo similar vascularization processes during development, it remains unknown how the surrounding vasculature, namely the arterial, venous, and lymphatic vessels, is assembled and patterned.
Prior studies have advanced our understanding of the cellular and molecular mechanisms governing CNS vascularization and have identified cells and factors that are important for CNS vascularization (Haigh et al., 2003; Raab et al., 2004; Xu et al., 2004; Proctor et al., 2005; Stenman et al., 2008; Daneman et al., 2009; Ye et al., 2009; Junge et al., 2009; Kuhnert et al., 2010; Ma et al., 2013; Whiteus et al., 2014; Lacoste et al., 2014; Okabe et al., 2014; Zhou et al., 2014; Arnold et al., 2014; Takahashi et al., 2015; Vanhollebeke et al., 2015). Neuronal progenitors, including neuroepithelial cells and radial glia, play critical roles in the ingression of blood vessels into neural tissues (Haigh et al., 2003; Raab et al., 2004; Stenman et al., 2008; Daneman et al., 2009), as well as their stabilization in the cerebral cortex (Ma et al., 2013). Although it has been clearly shown that the ingression of blood vessels into neural tissues occurs through angiogenic sprouting from the PNVP in different organisms (Kurz et al., 1996; Hogan et al., 2004; James et al., 2009; Takahashi et al., 2015), and that the developing neural tube provides signals to recruit the endothelial cells (ECs) that form the PNVP (Chapman and Papaioannou, 1998; Hogan et al., 2004), how arterial and venous vessels are assembled around the CNS remains unclear. The terminals, or end-feet, of neuronal progenitors lie in close proximity to blood vessels in the basal lamina at the surface of the developing CNS (Halfter et al., 2002; Kriegstein and Alvarez-Buylla, 2009; Lam et al., 2009; Vallon et al., 2014; Nakagawa et al., 2015), raising the possibility that these cells are involved in regulating vascular development around the CNS. However, the role of the different CNS cell types in regulating the vascular architecture around the CNS remains to be investigated.
To systematically determine the extent to which different CNS cell types control vascular development around the CNS, we utilized the zebrafish larva as a model system as its optical clarity allows the easy visualization of its stereotyped yet simple vascular pattern (Isogai et al., 2001). In addition, the use of an established genetic cell ablation method that utilizes the bacterial enzyme Nitroreductase (NTR) to induce apoptotic cell death upon administration of its substrate prodrug metronidazole (Mtz) (Curado et al., 2007; Pisharath et al., 2007; Curado et al., 2008) allowed us to ablate different CNS cell types in a spatially and temporally controlled manner. In combination with genetic mutants and pharmacological tools, we used this ablation technology to analyze the roles of distinct CNS cell types in patterning the vasculature around the spinal cord.
As the developing zebrafish CNS is known to be composed of different glial and neuronal cell types, we first categorized them into major cell type groups: radial glia neuronal progenitors, neurons, oligodendrocytes, and microglia. Unlike in the mammalian CNS, radial glia neuronal progenitors persist into adulthood in many regions of the zebrafish CNS (Lam et al., 2009; Than-Trong and Bally-Cuif, 2015); and to date, there is no clear evidence for bona fide astrocytes in the developing zebrafish CNS at embryonic or early larval periods, the stages we analyzed in this study.
Prior to ablating these different cell types, we first conducted an extensive analysis of potential interaction sites where the vasculature and cell bodies and/or processes from these CNS cell types are physically adjacent at different developmental stages. Through these analyses, we identified that cellular processes marked by TgBAC(gfap:Gfap-EGFP)zf167 expression lie in close proximity to different vessels in the trunk, including intersegmental vessels (ISVs) and the vertebral arteries (VTAs) (Figure 1A–C’). TgBAC(gfap:Gfap-EGFP) expression prominently and almost exclusively marks one cell type in the developing spinal cord, one that extends long radial processes from the ventricular lumen towards the pial surface, a morphological feature that is characteristic of radial glia (Bernardos and Raymond, 2006; Lam et al., 2009; Than-Trong and Bally-Cuif, 2015) (Figure 1B–C’ and Video 1). Through careful analyses at different developmental stages, we also observed that the physical proximity between radial glia end-feet and ISVs as well as VTAs persists throughout development. These observations along with the fact that a similar arrangement can be seen in the developing mouse trunk (Vallon et al., 2014) motivated us to investigate the potential role of spinal cord radial glia in the development of these trunk vessels.
We thus started by ablating radial glia during development. In parallel, we also ablated neurons, since the role for neurons in vascular development around the CNS had not been systematically addressed. To ablate radial glia, we generated a new transgenic (Tg) line that drives Gal4ff under the control of the same gfap BAC promoter used for TgBAC(gfap:gfap-EGFP)zf167 (Lam et al., 2009). We confirmed that this newly generated TgBAC(gfap:gal4ff)s995 line indeed marks radial glia in the developing spinal cord by crossing it with the previously characterized Tg(gfap:GFP)mi2001 line (Bernardos and Raymond, 2006), as well as by performing immunohistochemistry using a pan-neuronal anti-HuC/HuD antibody (Figure 1D–E”). We then crossed TgBAC(gfap:gal4ff)s995 fish to Tg(UAS-E1b:Eco.NfsB-mCherry)c264 fish, which carry a NTR-mcherry fusion gene downstream of UAS (upstream activating sequence), in order to generate TgBAC(gfap:gal4ff)s995;Tg(UAS-E1b:Eco.NfsB-mCherry)c264 animals, hereafter abbreviated Tg(gfap:NTR). To ablate neurons, we used Tg(elavl3:gal4-vp16)psi1;Tg(UAS-E1b:Eco.NfsB-mCherry)c264 fish, hereafter abbreviated Tg(elavl3:NTR). We first tested and confirmed that these lines can induce radial glia or neuron ablation robustly upon administration of Mtz (Figure 1F–I” and Figure 1—figure supplement 1C–I”). Furthermore, we confirmed by acridine orange staining and TUNEL assays that these lines induce apoptotic cell death specifically in the CNS (data not shown), and that when we initiated cell ablation at 30 hpf, radial glia and neurons in the spinal cord are largely segregated as determined by the expression of fluorescent proteins driven by the gfap (Lam et al., 2009) and elavl3 (Park et al., 2000) promoters, respectively (Figure 1—figure supplement 1A and B).
We then investigated whether and how radial glia or neurons regulate vascular development around the CNS by crossing Tg(gfap:NTR) or Tg(elavl3:NTR) fish into the EC reporter Tg line, Tg(kdrl:EGFP)s843. To analyze the role of each cell type in vascular development, we performed the genetic ablation at early developmental stages. We set up an experiment where dechorionated embryos were treated with 2 mM Mtz starting at 30 hpf and assessed vascular patterning at 154 hpf (Figure 2A). We observed that radial glia-ablated fish exhibited largely comparable patterns of the trunk vasculature to controls; however, we found a severe vascular patterning defect in a specific region of radial glia-ablated trunks (Figure 2B and C; quantification shown in Figure 2F; n = 25 fish for each group). Namely, radial glia-ablated fish developed ectopically sprouting vessels between the ISVs in the dorsal part of the trunk adjacent to the spinal cord (Figure 2C and Video 2). These ectopic vessels were observed at the surface of, but not inside, the spinal cord (Video 2) and were not observed in control DMSO or 2 mM Mtz treated fish (Figure 2B; data not shown). Intriguingly, we also did not observe a similar vascular defect in neuron-ablated fish (Figure 2D and E; n = 25), suggesting a specific role for radial glia in regulating this aspect of trunk vascular patterning. Importantly, these observations also show that the cell responses evoked by massively-induced apoptotic cell death in the CNS are not sufficient to cause this vascular phenotype (Figure 2B–F). Thus, radial glia appear to function as negative angiogenic regulators during the patterning of dorsal ISVs around the spinal cord during development.
It is important to note that the vascular phenotypes after radial glia ablation are unlikely to be caused by the reduction or loss of other CNS or PNS cell types such as oligodendrocytes, microglia, or Schwann cells, since animals treated with cyclopamine, which leads to a dramatic loss of spinal cord oligodendrocytes and oligodendrocyte precursor cells, irf8st96 mutants, which lack microglia (Shiau et al., 2015), or erbb2st61 mutants, which have a reduced number of Schwann cells (Lyons et al., 2005), did not display these vascular phenotypes (Figure 3A–H). Furthermore, cell types such as macrophages, neutrophils, or pericytes, which play roles in angiogenesis and/or vascular remodeling (Gong and Koh, 2010; Ribatti et al., 2011; Newman and Hughes, 2012; Arnold and Betsholtz, 2013), are also unlikely to be involved; the use of mutants, including irf8st96, which lack microglia and have a dramatically reduced number of macrophages up to 5–6 dpf (Shiau et al., 2015), and pdgfrbum148, which have a reduced number of pericytes (Kok et al., 2015; Ando et al., 2016), as well as an ablation Tg line, Tg(mpx:gal4):Tg(UAS-E1b:Eco.NfsB-mCherry), which leads to a dramatically reduced number of neutrophils following cell ablation (data not shown), did not affect the severity of the vascular phenotypes after radial glia ablation (Figure 2—figure supplement 1; data not shown). Thus, these findings strongly suggest that specifically radial glia, but not other CNS-resident cell types including those derived from radial glia, regulate this vascular patterning process.
Identification of a specific role played by radial glia in trunk vascular patterning led us to further characterize the phenotype. We first determined whether the ectopic dorsal trunk vessels after radial glia ablation were caused by mis-migration or an increased number of ECs. For this purpose, we quantified the number of ECs that constitute the trunk vasculature using a Tg(kdrl:NLS-EGFP)ubs1 reporter line. We divided the trunk vasculature into dorsal and ventral parts for this quantification. We counted the number of ECs in the dorsal part, including the dorsal ISVs, the VTAs, and the dorsal longitudinal anastomotic vessels (DLAVs) and found an approximately 30% increase in EC numbers in radial glia-ablated fish compared to control or neuron-ablated fish (Figure 2G–K and Figure 2—source data 1; n = 6 for each group). In contrast, the number of ECs in the ventral part, where we counted ECs in ventral ISVs and the dorsal aorta (DA), did not differ between radial glia-ablated, neuron-ablated, and control fish (Figure 2G–K and Figure 2—source data 1; n = 6 for each group). These results show that radial glia ablation leads to ectopic sprouting and an increased number of ECs specifically in the dorsal trunk. Thus, these cell ablation experiments identify a unique role for CNS radial glia in regulating trunk vascular patterning around the spinal cord.
To gain mechanistic insight into how radial glia regulate trunk vascular patterning, we first characterized in detail the ectopic vessels that emerge after radial glia ablation. We analyzed the growth progression of the ectopic sprouts at different developmental stages of radial glia-ablated fish that were treated with Mtz between 30 and 54 hpf. Around 74 hpf, when a majority of radial glia were ablated, we observed ectopic vessel sprouting, and these ectopic vessels continued to grow until 6–7 dpf (Figure 3—figure supplement 1A–P; data not shown). Furthermore, by comparing radial glia-ablated fish that were treated with Mtz for different lengths of time, we found that the emergence of the ectopic vessels correlated with regions where radial glia were robustly ablated (Figure 3—figure supplement 1Q–W’), indicating that radial glia modulate nearby vessels to prevent their over-sprouting. To determine when radial glia regulate vascular patterning in the trunk, we ablated radial glia at different developmental stages. Ectopic vessel sprouting emerged only when we initiated radial glia ablation at early developmental stages, i.e., before 60 hpf, suggesting a critical developmental time window of negative angiogenic action of radial glia and/or the vessels’ response (data not shown).
We next assessed whether the ectopic vessels that emerged after radial glia ablation were arterial or venous using the Tg(-0.8flt1:tdTomato)hu5333 line, which has been reported to mark arterial ISVs strongly and venous ISVs weakly (Bussmann et al., 2010). The Tg(-0.8flt1:tdTomato) line indeed labeled arterial and venous ISVs differently in our hands as well, and this differential expression of tdTomato in aISVs versus vISVs became clear at 56 hpf and even more obvious at 80 hpf (Figure 3—figure supplement 2A–C”). By analyzing ectopic sprouts after radial glia ablation in 100 hpf Tg(-0.8flt1:tdTomato);Tg(kdrl:EGFP);Tg(gfap:NTR) fish, we found that a vast majority of the ectopic sprouts derived from vISVs (Figure 3I–K; 106 out of 110 sprouts derived from vISVs; n = 17 fish). In addition to this assessment by the differential tdTomato expression in aISVs versus vISVs, we also carefully examined ISVs’ connections with their axial vessels, namely the DA and posterior cardinal vein (PCV), and observed that the ectopic sprouts after radial glia ablation emerge selectively from vISVs as they were directly connected to the PCV (Figure 3I–J”). At 154 hpf, when the ectopic sprouts deriving from vISVs appeared to be more mature and integrate within the circulatory loop (Figure 3M and N), a majority of these ectopic vessels showed weak Tg(-0.8flt1:tdTomato) expression similar to that of vISVs (Figure 3L–L”), suggesting that these vessels are of venous identity.
To further test whether this effect of radial glia ablation is selective for vISVs, we performed experiments that genetically reduce the number of vISVs. If the effect of radial glia ablation is indeed specific for vISVs, reduction of their numbers should lead to a decrease in excessive vessel sprouting. To achieve this vISV reduction, we generated a Tg(hsp70l:sflt4, cryaa:cerulean) line, hereafter abbreviated Tg(hsp70l:sflt4), which upon heat shock overexpresses a soluble form of Flt4/Vegfr3 (sFlt4), a decoy receptor for Vegfc and Vegfd (Ruiz de Almodovar et al., 2009). This transgene also contains the eye-marker cassette, cryaa:cerulean (Kurita et al., 2003; Hesselson et al., 2009), to facilitate the identification of transgenic animals. Compromised Vegfc/Vegfr3 signaling was previously shown to cause a dramatically reduced number of vISVs as assessed in zebrafish vegfc and vegfr3 mutants (Hogan et al., 2009b; Le Guen et al., 2014). We found that overexpression of sFlt4 by heat shocking the embryos at 29, 36, and 43 hpf, stages when angiogenic sprouting from the PCV actively occurs, recapitulated these mutant phenotypes, resulting in a reduced number of vISVs (approximately 9% vISVs remaining per transgenic fish on average, Figure 4A,C,E, and Figure 4—source data 1; n = 23). Notably, when we performed radial glia ablation in these fish with a reduced number of vISVs, we found that the ectopic sprouting after radial glia ablation was dramatically reduced as compared to non-heat shocked or heat shocked control siblings (Figures 4B–D and F; n = 15 for each group), which have approximately 55% vISVs on average (Figure 4E and Figure 4—source data 1; n = 18). These results provide further evidence that radial glia ablation causes the excessive sprouting of venous ECs predominantly, and thus suggest that radial glia negatively regulate the over-sprouting of dorsal trunk venous vessels during development.
To determine which angiogenic signal(s) triggers ectopic vessel sprouting after radial glia ablation, we used pharmacological and genetic tools that inhibit different angiogenic signaling pathways. We first used small molecule inhibitors to identify signaling pathways responsible for the ectopic vessel sprouting. Specifically, we treated embryos which were pre-incubated with 2 mM Mtz between 30 and 54 hpf, with the following chemicals from 54 until 130 hpf: 2 µM sunitinib, a broad receptor tyrosine kinase inhibitor, 2.5 µM SKLB1002, a selective Vegfr2 inhibitor, 10 µM LY294002, a selective PI3 kinase inhibitor, 5 µM DMHI, a selective Bmp receptor inhibitor, 15 µM AG1295, a selective Pdgf receptor inhibitor, and 3 µM PD158780, a selective ErbB receptor tyrosine kinase inhibitor. Among the chemicals tested, selective inhibitors for Bmp, Pdgf, or ErbB receptors did not block ectopic vessel sprouting after radial glia ablation (Figure 4K; n = 13–17 for each treatment group), suggesting that these signaling pathways are not required for inducing the ectopic vessel sprouting. In contrast, inhibitors for receptor tyrosine kinases (sunitinib), Vegfr2 (SKLB1002), and PI3 kinase (LY294002) significantly blocked ectopic vessel sprouting, indicating that the Vegfr2 signaling pathway is responsible for the phenotype observed after radial glia ablation (Figure 4G–K; n = 16 for each treatment group).
To further test these hypotheses, we also used genetic tools that block the Pdgf, Bmp, or Vegf signaling pathways. Consistent with the chemical treatment results, neither the pdgfrbum148 mutants nor overexpression of the BMP inhibitor Noggin3 using Tg(hsp70l:nog3)fr14 fish (Chocron et al., 2007), blocked the ectopic vessel sprouting after radial glia ablation (Figure 2—figure supplement 1E–H and Figure 4—figure supplement 1A–E; n = 11 for pdgfrb-/- fish and n = 24 for Tg(hsp70l:nog3) fish with multiple heat shocks). To investigate which Vegf ligand(s) and receptor(s) are responsible for inducing the ectopic vessel sprouting after radial glia ablation, we generated and used a Tg(hsp70l:sflt1, cryaa:cerulean) line, hereafter abbreviated Tg(hsp70l:sflt1), which upon heat shock overexpresses a soluble form of Flt1/Vegfr1 (sFlt1), a decoy receptor for Vegfa, Vegfb, and PIGF (Placental growth factor) (Ruiz de Almodovar et al., 2009), as well as the Tg(hsp70l:sflt4) line as described earlier (Figure 3—figure supplement 2D–S). We found that ectopic vessel sprouting after radial glia ablation was dramatically blocked in Tg(hsp70l:sflt1) but not Tg(hsp70l:sflt4) fish, after heat shocking the animals every 12 hr starting at 62 hpf, a stage prior to the onset of ectopic vessel sprouting (Figure 4—figure supplement 1F–H). Therefore, these results indicate that ectopic vessel sprouting after radial glia ablation is dependent on Vegfr2, but not Vegfr3, signaling. Consistent with the chemical treatment results, these findings identify Vegf/Vegfr2 signaling as a critical signaling pathway responsible for ectopic vessel sprouting after radial glia ablation, indicating that radial glia negatively modulate this signaling pathway during trunk vasculature development.
An endogenous protein that is known to act as a negative regulator of Vegf/Vegfr2 signaling is sFlt1. Previous studies have shown that sFlt1 functions as a Vegf decoy receptor and thereby limits angiogenic sprouting induced by Vegf/Vegfr2 signaling (Ruiz de Almodovar et al., 2009). We thus hypothesized that radial glia negatively modulate Vegf/Vegfr2 signaling via sFlt1 to prevent vISV over-sprouting. To test this hypothesis, we generated zebrafish sflt1 mutants by targeted genome editing using the CRISPR/Cas9 system (Figure 5A,B, and Figure 5—figure supplement 1). We identified a mutation, bns29, which is predicted to lead to a premature stop codon at tyrosine residue 86 of both sFlt1 and a membrane-bound form of Flt1/Vegfr1 (mFlt1) (Figures 5A and Figure 5—figure supplement 1). We also used flt1fh390 mutants, which are predicted to lack the transmembrane and tyrosine kinase domains of mFlt1 without affecting sFlt1 (Rossi et al., 2016), in order to determine the role of mFlt1. The genotypes of flt1bns29 and flt1fh390 animals were determined by high resolution melt analysis (Figure 5B). Interestingly, we observed that the flt1fh390 mutants, which lack mFlt1 signaling function, do not exhibit any obvious vascular phenotypes in the trunk (Figure 5I; n = 20). However, we found that the flt1bns29 mutants, which lack sFlt1 function, exhibit ectopic vessel sprouting specifically around the spinal cord (Figure 5C–J; n = 20–24 for each genotype), a phenotype similar to that found after radial glia ablation. Thus, phenotypic analyses of these different flt1 mutants suggest that sFlt1, but not mFlt1, functions to prevent excessive sprouting of ISVs in the dorsal trunk. In addition, we found that ectopic vessel sprouting in flt1bns29 mutants begins around 74 hpf, and that these ectopic vessels mostly derive from vISVs, as observed after radial glia ablation. As assessed by Tg(-0.8flt1:tdTomato) expression, ectopic sprouts in flt1bns29 mutants mostly derive from vISVs at 100 hpf (Figure 5K–K”) and at 154 hpf exhibit weak Tg(-0.8flt1:tdTomato) expression as vISVs do (Figure 5L–L”), which is again very similar to what was observed after radial glia ablation.
To gain mechanistic insight into how radial glia and sFlt1 may cooperate to regulate this vascular patterning, we first characterized sFlt1 expression in detail. Previous work has shown sflt1 expression primarily in ECs during early embryonic stages by in situ hybridization (Krueger et al., 2011; Zygmunt et al., 2011), and has also reported sflt1 and/or mflt1 expression in some neurons within the spinal cord by analyzing a BAC transgenic reporter line, TgBAC(flt1:YFP)hu4624, in which YFP is inserted in a flt1 BAC (Hogan et al., 2009a). We first carefully examined TgBAC(flt1:YFP) expression at stages when ectopic sprouting emerges in flt1bns29 mutants, and observed that TgBAC(flt1:YFP) expression is indeed found in the vasculature as well as in some spinal cord cells (Figure 6A and A’). As suggested previously (Krueger et al., 2011), we observed that this TgBAC(flt1:YFP) expression within the spinal cord is in neurons, since genetic ablation of neurons resulted in an almost complete loss of this expression (Figure 6A–B’). In addition, we found that TgBAC(flt1:YFP) expression within the spinal cord did not co-localize with the radial glia mCherry reporter expression at 82 hpf (Figure 6C–D”; none of 51 TgBAC(flt1:YFP)-positive cells analyzed in 6 fish were positive for the radial glia mCherry reporter), suggesting that radial glia are unlikely to be a source of sFlt1 or mFlt1.
In order to address the cell-autonomy of sFlt1 function in patterning the veins around the spinal cord, we transplanted flt1bns29 mutant cells with a GFP endothelial label, TgBAC(etv2:EGFP)ci1, or flt1+/+ cells with a BFP endothelial label, Tg(kdrl:tagBFP)mu293, into WT or sflt1 mutant animals, respectively (Figure 6E). We found that when flt1bns29 mutant cells were transplanted into flt1+/+ hosts, some transplanted mutant ECs, but not flt1+/+ ECs, exhibited ectopic sprouting (Figure 6F,G, and J; 79 out of 179 transplanted dorsal ISVs exhibited ectopic sprouting in 31 fish analyzed). Conversely, when flt1+/+ cells were transplanted into flt1bns29 mutant hosts, most transplanted flt1+/+ ECs did not show ectopic sprouting, in contrast to flt1bns29 mutant ECs that exhibited clear sprouting (Figure 6H,I, and J; 137 out of 144 transplanted dorsal ISVs exhibited no ectopic sprouting in 33 fish analyzed). Thus, these transplantation data indicate that sFlt1 acts cell-autonomously in endothelial cells to limit ectopic sprouting.
Based on the phenotypic similarities observed after radial glia ablation and in flt1bns29 mutants, we hypothesized that radial glia positively regulate sFlt1 function in vivo. We started to test this hypothesis by examining gene expression and performed qPCR analysis for sflt1 and the other Vegf receptor genes on cDNA obtained from 100 hpf Tg(gfap:NTR) fish trunk mRNA after treatment with DMSO or Mtz starting at 30 hpf. We found that sflt1 and mflt1, but not vegfr2 or vegfr3, expression was significantly reduced in the Mtz-treated animals (Figure 7A). In contrast, when we compared gene expression in 148 hpf Tg(gfap:NTR) trunk cDNA after treatment with DMSO or Mtz starting at 78 hpf, we did not find significant differences in sflt1 and mflt1 expression, as compared to controls (Figure 7B). These data are consistent with our observations that radial glia ablation in early embryos, but not in later larval stages (data not shown), leads to excessive sprouting of vISVs, and indicate that radial glia regulate sflt1 expression during embryonic stages. Given the previous reports that sflt1 is primarily expressed in ECs during embryonic stages (Krueger et al., 2011; Zygmunt et al., 2011), it is likely that radial glia regulate sflt1 expression in a cell non-autonomous manner.
We next asked whether the sflt1 mutation affected the sensitivity of vISVs after radial glia ablation by comparing vessel sprouting in flt1+/+ and flt1bns29/+ fish. We used a lower concentration of Mtz (50 µM) for these experiments to reduce the extent of ISV over-sprouting after radial glia ablation (Figure 7C; n = 23–30). Notably, we found that flt1bns29/+ fish exhibit a markedly increased degree of ISV over-sprouting after partial radial glia ablation as compared to controls (Figure 7C and Figure 7—source data 1; n = 33), providing evidence that radial glia ablation and sFlt1 functionally interact. We also found that overexpression of sFlt1, but not sFlt4, fully blocked the ectopic ISV sprouting after radial glia ablation, thereby normalizing vascular patterning around the spinal cord (Figure 7D–H; n = 20 for each group). These findings show that sFlt1 overexpression is sufficient to rescue the ectopic vISV sprouting phenotype after radial glia ablation, and suggest that sFlt1 acts downstream of radial glia in the regulation of this vascular patterning process.
In this work, we identified previously unrecognized, yet critical, roles for CNS-resident progenitors in orchestrating the vascular architecture around the CNS. Our findings reveal that radial glia within the CNS act as negative as well as selective angiogenic regulators that determine the precise patterning of the venous vasculature around the developing spinal cord (Figure 7I). Specifically, we found that radial glia ablation in zebrafish embryos leads to the over-sprouting of venous ISVs around the spinal cord, a process driven by Vegf/Vegfr2 signaling; we also found that sflt1 mutants recapitulate the vascular phenotype observed after radial glia ablation, and that sFlt1 acts downstream of radial glia and functions in endothelial cells to limit venous over-sprouting around the spinal cord. Altogether, these findings suggest a model whereby radial glia positively regulate sFlt1 function in endothelial cells to establish the precise venous patterning around the spinal cord during embryonic and early larval development, providing critical and novel insights into the cellular and molecular mechanisms by which the vascular networks around developing organs are patterned.
Many questions emerge from these findings. First, we speculate that the regulation of vascular patterning around the developing CNS by radial glia may constitute a means to ensure optimal vascularization for CNS function, and thus, determining the functional relevance of the observed vascular defects is one of the critical next steps. These findings indicate more generally that progenitor cells in developing organs may function as critical regulators to establish the microenvironment for the mature organs derived from these progenitors. Second, it will be of particular interest to the neuroscience and vascular biology fields to further investigate how CNS radial glia differentially modulate arterial and venous ECs. Recent studies have discovered a lymphatic network lining the meningeal dura mater of the mouse brain (Aspelund et al., 2015; Louveau et al., 2015), and whose architecture is very distinct from that of the arterial and venous networks in the CNS. Our identification of spinal cord radial glia as negative as well as selective angiogenic regulators that specifically affect venous vessels is intriguing in light of previous studies that revealed neuronal progenitors as positive angiogenic regulators that initiate arterial sprouting into neural tissues (Kurz et al., 1996; Haigh et al., 2003; Kurz, 2009). These findings may indicate that CNS-resident progenitors are able to differentially regulate the patterning of these distinct vessel networks within as well as around the CNS.
How do CNS radial glia and sFlt1 selectively regulate venous ECs around the developing spinal cord? One hypothesis is that the distinct density and/or characteristics of perivascular cells that cover arteries and veins play a role in this process. Indeed, it was recently shown that in zebrafish, mural cells emerge around the ISVs starting at 48 hpf and that they preferentially cover aISVs (Ando et al., 2016). Preferential coverage of arteries by mural cells was also observed in mouse embryos (Hellstrom et al., 1999). This differential coverage of arterial and venous ISVs by mural cells may explain the near exclusive over-sprouting of vISVs after radial glia ablation and in sflt1 mutants. Perhaps, coverage of aISVs by mural cells blocks most communication between radial glia and arterial ECs. To begin to test this hypothesis, we carefully analyzed pdgfrbum148 mutants (Kok et al., 2015), which should exhibit a slightly decreased number of ISV-covering mural cells as previously shown in pdgfrbsa16389 mutants (Ando et al., 2016), after ablating radial glia starting at 30 hpf. However, we did not observe a significantly increased number of over-sprouting aISV in these experiments (data not shown). We speculate that apparently decreased, yet incompletely eliminated, ISV-covering mural cells in these pdgfrb mutant animals (Kok et al., 2015; Ando et al., 2016) could still protect aISVs from over-sprouting after radial glia ablation. Alternative approaches that allow complete ablation of ISV-covering mural cells will be needed to address this issue in a more conclusive manner.
How do radial glia regulate sflt1 expression? Previous work indicates that Sema/PlxnD1 signaling positively regulates sflt1 expression in zebrafish embryos (Zygmunt et al., 2011). It was shown that sflt1 transcripts detected with a sflt1-specific riboprobe were markedly decreased in plxnd1fov01b mutants and that sflt1 transcript levels measured by qPCR were also reduced in plxnd1fov01b/+ embryos compared to WT (Zygmunt et al., 2011). Although we did not observe ectopic sprouting from the DA in flt1bns29 mutants as was seen in plxnd1fov01b mutants (Zygmunt et al., 2011), it is still possible that this signaling pathway mediates the negative angiogenic effects of radial glia and regulates sflt1 expression to limit venous over-sprouting around the spinal cord. Continuous overexpression of dominant-negative PlxnD1 in ECs from late embryonic stages (around 2.5 dpf) may allow us to test this hypothesis. Regarding sFlt1 function, our genetic mosaic analyses show that sFlt1 function in ECs can limit venous over-sprouting around the spinal cord. However, TgBAC(flt1:YFP) expression is also observed in small subsets of spinal cord neurons (Figure 6A–B’)(Krueger et al., 2011). Although we did not observe vISV over-sprouting in neuron-ablated fish (Figure 2D–F), which show a loss of TgBAC(flt1:YFP) expression in the spinal cord (Figure 6A–B’), it is possible that Flt1 in spinal cord neurons may also contribute to the vISV over-sprouting phenotype observed in flt1bns29 mutants. Finally, whether the communication between radial glia and venous ECs involves secreted factors and/or direct cell-cell communication remains a major question to resolve.
In summary, our observations of vascular pattern regulation within mesodermal tissues by adjacent ectoderm-derived CNS radial glia suggest a mechanism by which tissue vascularization is coordinated by adjacent tissue interactions. The interaction between factors generated by the ectoderm and factors deriving from resident cells in the mesoderm opens a new avenue for future studies on the coordination of tissue vascularization; and it will be of broad interest to determine whether and how vascularization events between different tissues (e.g., endoderm-derived organs and mesodermal tissues) are coordinated during development. Therefore, our identification of a critical role for CNS-resident progenitors in patterning the vasculature around the CNS will advance our understanding of the mechanisms governing vascular network formation, in particular how distinct vessel networks, as well as vascularization patterns, around developing organs are formed.
All zebrafish husbandry was performed under standard conditions in accordance with institutional (UCSF and MPG) and national ethical and animal welfare guidelines. Tg(kdrl:EGFP)s843 (Jin et al., 2005), Tg(kdrl:NLS-EGFP)ubs1 (Blum et al., 2008), Tg(kdrl:Has.HRAS-mcherry)s896 (Chi et al., 2008), Tg(fli1a:EGFP)y1 (Lawson and Weinstein, 2002), TgBAC(etv2:EGFP)ci1 (Proulx et al., 2010), Tg(-0.8flt1:tdTomato)hu5333 (Bussmann et al., 2010), TgBAC(flt1:YFP)hu4624 (Hogan et al., 2009a), Tg(elavl3:gal4-vp16)psi1 (Stevenson et al., 2012), TgBAC(gfap:gfap-gfp)zf167 (Lam et al., 2009), Tg(gfap:GFP)mi2001 (Bernardos and Raymond, 2006), Tg(elavl3:EGFP)knu3 (Park et al., 2000), Tg(UAS-E1b:NfsB-mCherry)c264 (Davison et al., 2007), Tg(mpx:gal4)sh267 (Robertson et al., 2014), Tg(-4.9sox10:EGFP)ba2 (Carney et al., 2006), Tg(hsp70l:nog3)fr14 (Chocron et al., 2007), irf8st96 (Shiau et al., 2015), pdgfrbum148 (Kok et al., 2015), erbb2st61 (Lyons et al., 2005), and flt1fh390 (Rossi et al., 2016) were used in this study. Fish embryos/larvae were raised at 28°C.
A TgBAC(gfap:gal4ff)s995 fish line was generated by following the standard BAC recombineering protocol described previously (Bussmann and Schulte-Merker, 2011). Briefly, the CH211-154O10 BAC clone (BACPAC Resource Center) was engineered to replace the gfap start codon with gal4ff. The engineered construct was injected into one-cell stage embryos together with transposase mRNA transcribed in vitro. The Tg(hsp70l:sflt1, cryaa-cerulean)bns80 and Tg(hsp70l:sflt4, cryaa-cerulean)bns82 fish lines were generated by inserting zebrafish sflt1 and human sFLT4-IgG-Fc (Makinen et al., 2001), respectively, under the zebrafish hsp70l promoter (Halloran et al., 2000). The eye-marker cassette, cryaa:cerulean (Kurita et al., 2003; Hesselson et al., 2009), was also introduced in the same construct. These constructs were then injected into one-cell stage embryos together with I-Sce I meganuclease (NEB) supplemented with 1X cutsmart NEB buffer. The Tg(kdrl:tagBFP)mu293 fish line was generated by cloning the sequence encoding tagBFP downstream of a 7.6 kb kdrl promoter flanked by tol2 sites. kdrl:tagBFP plasmid DNA was injected together with transposase mRNA.
The flt1bns29 mutant allele was generated by targeted genome editing using the CRISPR/Cas9 system as follows: We targeted the third exon of flt1, which encodes part of the 1st Ig-like domain. The flt1bns29 mutant allele harbors a 1 base pair deletion and a 3 base pair insertion. The flt1bns29 allele (c.258delinsGGC) is predicted to lead to a premature stop codon at tyrosine residue 86 and thus encode a truncated polypeptide containing a stretch of 85 amino acids of both sFlt1 and mFlt1. The Cas9 vector (pT3TS-nlsCas9nls) was purchased from Addgene. Cas9 mRNA was prepared in vitro using the mMESSAGE mMACHINE T3 transcription kit (Ambion) after linearizing the plasmid with XbaI (NEB). The mRNA was purified using RNA Clean & Concentrator-5 kit (Zymo Research). The gRNA was designed using Optimized CRISPR Design algorithm (http://crispr.mit.edu). The oligos (taggGTGTCAGCCGGCTGCAATAC and aaacGTATTGCAGCCGGCTGACAC) were annealed and ligated into the gRNA plasmid (pT7-gRNA vector) after digesting the plasmid with BsmbI (NEB). The gRNA was prepared in vitro using the MEGAshortscript T7 transcription kit (Ambion) after linearizing the plasmid with BamHI-HF (NEB). The gRNA was purified using RNA Clean & Concentrator-5 kit. 1 nL of a solution containing 250 ng/µl of Cas9 mRNA and 100 ng/µl of gRNA was injected at the one-cell stage.
WT, heterozygous, and homozygous flt1bns29 or flt1fh390 animals were identified by high-resolution melt analysis of PCR using the following primers:
flt1 bns29 Fw: 5’- ACTCAGTGCGGGAAGAAAAG -3’
flt1 bns29 Rv: 5’- CCCGTGTGCTGAGTTAAAGC -3’
flt1 fh390 Fw: 5’- CAGTTGAAGACCAGGGATTTT -3’
flt1 fh390 Rv: 5’- CCACAGACCCCCTCTGATT -3’
An Eco Real-Time PCR System (Illumina) was used for the PCR reactions and high-resolution melt analysis. DyNAmo SYBR green (Thermo Fisher Scientific, Germany) was used in these experiments. PCR reaction protocols were 95°C for 15 s, then 40 cycles of 95°C for 2 s, 60°C for 2 s, and 72°C for 2 s. Following the PCR, a high-resolution melt curve was generated by collecting SYBR-green fluorescence data in the 65–95°C range. The analyses were performed on normalized derivative plots.
Mtz substrate (Sigma, M3761) was used at 2 mM dissolved in egg water containing 1% DMSO for most of the cell ablation experiments in this study. Prior to treatment with 2 mM Mtz or 1% DMSO control, embryos were manually dechorionated with forceps and then incubated with freshly prepared 2 mM Mtz or 1% DMSO in egg water. To wash away the Mtz, fish embryos/larvae were washed twice in dishes containing egg water. Although a minority of the animals developed prominent pericardial edema and/or severe gross anatomical abnormalities after radial glia or neuronal ablation, most did not exhibit such abnormalities except non-inflated swim bladders and bent tails. We analyzed only the animals that did not exhibit pericardial edema or severe gross anatomical abnormalities. Treatment of flt1+/+ and flt1bns29/+ fish with Mtz was performed as follows: animals were treated with 50 µM Mtz or 1% DMSO between 30 and 154 hpf after manual dechorionation.
qPCR was performed on cDNA obtained from TgBAC(gfap:gal4ff)s995;Tg(UAS-E1b:NfsB-mCherry)c264 larval trunk mRNA after treatment with 1% DMSO or 2 mM Mtz. Animals were treated with 1% DMSO or 2 mM Mtz between 30 and 100 hpf or between 78 and 148 hpf. An Eco Real-Time PCR System was used for qPCR experiments, and gene expression levels were normalized relative to that of a reference gene, elfα. All reactions were performed in technical duplicates, and the results represent 4 independent biological samples (15 larval trunks pooled for each sample) including the SEM. Table 1 shows the primers used for these experiments.
An LSM 700 confocal laser scanning microscope (Zeiss) was used for live and immunofluorescence imaging. Fish embryos and larvae were anaesthetized with a low dose of tricaine, placed in a glass-bottom Petri dish (MatTek) with a layer of 1.2% low melt agarose, and imaged using W N-ACP 20X/0.5 and W Plan-Apochromat 40×/1.0 objective lenses. Immunostained fish sections were imaged using a C Apo 40X/1.1 objective lens. For FITC-Dextran microangiography, fluorescein isothiocyanate (FITC)-dextran, 2000 kDa (Sigma) was injected into the common cardinal vein and imaged after 10 min. An SMZ 25 stereomicroscope (Nikon) was used for brightfield images of anaesthetized fish.
Fish embryos/larvae raised at 28°C were subject to 37°C heat shock for 1 hr by replacing the egg water with pre-warmed (37°C) egg water and then kept in a 37°C incubator. After each heat shock, the fish embryos/larvae were kept at room temperature for 10 min to cool down and then transferred to a 28°C incubator. Heat shock experiments after radial glia ablation were performed as follows: TgBAC(gfap:gal4ff)s995;Tg(UAS-E1b:NfsB-mCherry)c264;Tg(kdrl:EGFP)s843;Tg(hsp70l:sflt1, cryaa-cerulean)bns80 and TgBAC(gfap:gal4ff)s995;Tg(UAS-E1b:NfsB-mCherry)c264;Tg(kdrl:EGFP)s843;Tg(hsp70l:sflt4, cryaa-cerulean)bns82 animals were treated with 2 mM Mtz between 30 and 54 hpf, washed twice in egg water, and then subject to one heat shock every 12 hr starting at 62 until 154 hpf. Heat shock experiments that reduce the number of vISVs were performed as follows: TgBAC(gfap:gal4ff)s995;Tg(UAS-E1b:NfsB-mCherry)c264;Tg(kdrl:EGFP)s843;Tg(hsp70l:sflt4, cryaa-cerulean)bns82 animals were given a heat shock at 29 hpf, then treated with 2 mM Mtz starting at 30 hpf. Mtz-treated fish embryos were then heat shocked at 36 and 43 hpf for 1 hr by transferring the dishes containing a 2 mM Mtz solution from a 28°C incubator to a 37°C incubator. After the heat shock at 43 hpf, the embryos were treated with freshly prepared 2 mM Mtz until 100 hpf, washed twice in egg water, and then analyzed at 154 hpf.
Pharmacological experiments after radial glia ablation were performed as follows: TgBAC(gfap:gal4ff)s995;Tg(UAS-E1b:NfsB-mCherry)c264; Tg(kdrl:EGFP)s843 embryos were treated with 2 mM Mtz between 30 and 54 hpf, washed twice in dishes containing egg water, and then treated with pharmacological inhibitors from 54 until 130 hpf, replacing the drug solution every 24 hr. Final concentrations of the chemicals used were as follows: 2 µM sunitinib (Sigma), 2.5 µM SKLB1002 (Calbiochem), 10 µM LY294002 (Calbiochem), 5 µM DMHI (Calbiochem), 15 µM AG1295 (Calbiochem), and 3 µM PD158780 (Tocris). All listed chemicals were first prepared as 100X stock solutions dissolved in 100% DMSO and then diluted 100 times in egg water shortly before use.
Cells were taken from TgBAC(etv2:EGFP)ci1 flt1bns29/bns29 or Tg(kdrl:tagBFP)mu293 flt1+/+ donor embryos at midblastula stages and transplanted into host embryos of the same age. Hosts were then imaged and analyzed at 154 hpf. For quantification, transplanted ECs that contributed to dorsal ISVs were analyzed for the presence of ectopic sprout(s) (each dorsal ISV that contained at least one transplanted EC was defined as a transplanted dorsal ISV). Note that when TgBAC(etv2:EGFP) flt1bns29/bns29 cells were transplanted into Tg(kdrl:tagBFP) flt1+/+ host embryos, we observed that approximately 5% of the transplanted hosts exhibited some mosaic EGFP expression in their spinal cord since TgBAC(etv2:EGFP)ci1 animals display non-specific EGFP expression in the neural tube of their trunk and tail (Proulx et al., 2010). We did not use animals with spinal cord EGFP expression in order to focus the analysis on ECs.
Tg(kdrl:EGFP)s843 or TgBAC(etv2:EGFP)ci1 EC reporter fish were used to quantify ectopic sprouts throughout this study. For the quantification of ectopic sprouts after radial glia or neuronal ablation, Tg(kdrl:EGFP)s843 fish were crossed to TgBAC(gfap:gal4ff)s995;Tg(UAS-E1b:NfsB-mCherry)c264 or Tg(elavl3:gal4-vp16)psi1;Tg(UAS-E1b:NfsB-mCherry)c264 fish, respectively. The 11 ISVs directly anterior to the anal opening were used for quantification (defined as 10 somites), and the number of somites that showed ectopic blood vessels in either side of the body was quantified and averaged.
Tg(kdrl:NLS-EGFP)ubs1 reporter fish were used to quantify EC number throughout this study. For the quantification of EC number after radial glia or neuronal ablation, Tg(kdrl:NLS-EGFP)ubs1 fish were crossed to TgBAC(gfap:gal4ff)s995;Tg(UAS-E1b:NfsB-mCherry)c264 or Tg(elavl3:gal4-vp16)psi1;Tg(UAS-E1b:NfsB-mCherry)c264 fish, respectively. The 5 ISVs directly anterior to the anal opening in both sides of the body were used to quantify the number of ECs in the dorsal and ventral parts of the trunk. Confocal z-stack images that span the ISVs in both sides of the body were taken, and cell numbers were manually determined using the ImageJ plugins.
Quantification of ectopic sprouts that derive from aISVs or vISVs after radial glia ablation was performed as follows: TgBAC(gfap:gal4ff)s995;Tg(UAS-E1b:NfsB-mCherry)c264; Tg(kdrl:EGFP)s843;Tg(-0.8flt1:tdTomato)hu5333 animals were treated with 2 mM Mtz between 30 and 100 hpf and then analyzed under the LSM 700 confocal microscope using a W Plan-Apochromat 40×/1.0 objective lens. Assignment of ectopic sprouts deriving from aISVs or vISVs was based on Tg(-0.8flt1:tdTomato) differential expression in aISVs and vISVs. As previously described (Bussmann et al., 2010), ISVs that were strongly labeled by Tg(-0.8flt1:tdTomato) expression were judged as aISVs, whereas those weakly labeled were judged as vISVs. In addition to using this differential Tg(-0.8flt1:tdTomato) expression between aISVs and vISVs, the identity of aISVs and vISVs was further confirmed by examining their connections with axial vessels, namely the dorsal aorta and posterior cardinal vein, respectively. The 11 ISVs directly anterior to the anal opening were used for quantification.
To analyze TgBAC(flt1:YFP)-positive spinal cord cells, TgBAC(flt1:YFP)hu4624 reporter fish were crossed to TgBAC(gfap:gal4ff)s995;Tg(UAS-E1b:NfsB-mCherry)c264 fish. High magnification single-plane confocal images of 80 hpf TgBAC(flt1:YFP)hu4624;TgBAC(gfap:gal4ff)s995;Tg(UAS-E1b:NfsB-mCherry)c264 spinal cords were taken using a W Plan-Apochromat 40×/1.0 objective lens and analyzed for the co-localization of YFP+ spinal cord cells and mCherry+ radial glia. To analyze TgBAC(flt1:YFP) expression after radial glia or neuronal ablation, TgBAC(flt1:YFP)hu4624 fish were crossed to TgBAC(gfap:gal4ff)s995;Tg(UAS-E1b:NfsB-mCherry)c264 or Tg(elavl3:gal4-vp16)psi1;Tg(UAS-E1b:NfsB-mCherry)c264 fish, respectively. Animals were treated with 1% DMSO or 2 mM Mtz between 30 and 82 hpf, and imaged at 82 hpf. After radial glia ablation, no obvious differences in YFP expression were observed.
Immunohistochemistry was performed as previously described (Matsuoka et al., 2011). The following primary antibodies were used: chicken anti-GFP (Aves Labs at 1:1000), rabbit anti-DsRed (Clontech at 1:300), and mouse anti-HuC/HuD (Invitrogen at 1:200).
Statistical differences for mean values among multiple groups were determined using a one-way analysis of variance (ANOVA) followed by Tukey's multiple comparison test. Statistical differences for mean values between two groups were determined using Student’s t-test. The criterion for statistical significance was set at p<0.05. Error bars are SEM.
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Marianne BronnerReviewing Editor; California Institute of Technology, United States
In the interests of transparency, eLife includes the editorial decision letter and accompanying author responses. A lightly edited version of the letter sent to the authors after peer review is shown, indicating the most substantive concerns; minor comments are not usually included.
Thank you for submitting your article "Radial Glia Regulate Vascular Patterning Around the Developing Spinal Cord" for consideration by eLife. Your article has been reviewed by three peer reviewers, and the evaluation has been overseen by Marianne Bronner as the Senior Editor and Reviewing Editor. The following individuals involved in review of your submission have agreed to reveal their identity: Naoki Mochizuki (Reviewer #2); Yoshiko Takahashi (Reviewer #3).
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In this manuscript, Matsuoka et al. identify a previously unappreciated mechanism in which radial glia repress venous sprouting around the spinal cord. Employing a variety of genetic tools in zebrafish, they demonstrate that ablation of radial glia leads to excessive venous sprouting, that this excessive sprouting requires Vegfr/Vegfr2 signaling, and that the normal repression of excessive venous sprouts is dependent on sFlt1 function within venous cells. The experiments are well-designed, the data are nicely presented, and the interpretation of the results is clear-cut. The implication of sFlt1 as a repressor of vascular sprouting in this context is consistent with previous work on sFlt1 function in other settings. The particular significance of this work comes from its novel demonstration that radial glia play an important role in patterning the CNS vascular network.
Several major questions regarding the repression of venous sprouting by radial glia remain unanswered by the experiments presented here:
1) The authors conclude that radial glia have a positive influence on the levels of sFlt1 expression, and they imply that local contacts between radial glia and venous cells could mediate this influence. The mechanism through which radial glia promote sFlt1 expression remains unaddressed, and the authors even refrain from speculating regarding this mechanism in the Discussion section. What are possibilities for this mechanism, based on what is already known about the regulation of sFlt1? For example, have the authors considered whether a Semaphorin-Plexin interface could influence sFlt1 expression in this context, as has been previously shown in the context of the dorsal aorta (Zygmunt et al., 2011)? Identification of this (or any other) molecular link between radial glia and venous cells would enhance the value of the authors' model; discussion of possible molecular links would enhance the scholarly value of the manuscript.
2) It is clear that the effects of radial glia are highly selective: excess venous sprouting is abundant following radial glia ablation, but excess arterial sprouting is almost never observed. The impact of this work would be enhanced by a better understanding of the mechanism for this selectivity. In the Discussion, the authors suggest the possibility that mural cells might protect arterial cells from the influence of radial glia. Is it possible to begin to test this idea, using mutations or ablation alleles that disrupt mural cell coverage? For example, pdgfrb-/- larvae presumably lack pericytes, so if pericyte coverage accounts for the difference in arterial and venous sprouting, then it might be possible to observe sprouting from aISVs in pdgfrb mutants. However, Figure 3F clearly shows no branching from aISVs. Can the authors explain this apparent inconsistency and discuss why aISVs are not affected? The presence of mural cells does not account for the difference between aISVs and vISVs.
3) In Figure 6, it looks as if Flit1 is also positive in aISV. If so, why does radial glia ablation affect only vISV and not aISV?https://doi.org/10.7554/eLife.20253.021
- Ryota L Matsuoka
- Ryota L Matsuoka
- Ryota L Matsuoka
- Ryota L Matsuoka
- Ryota L Matsuoka
- Didier YR Stainier
- Didier YR Stainier
- Didier YR Stainier
The funders had no role in study design, data collection and interpretation, or the decision to submit the work for publication.
We thank Herwig Baier, Cecilia Moens, William Talbot, and Stefan Schulte-Merker for kindly providing us with fish lines, Kari Alitalo for the human sFLT4-IgG-Fc plasmid, Ferdinand le Noble for discussions, Radhan Ramadass for help with the imaging, Petra Neeb and Rebecca Lee for technical assistance, Arica Beisaw, Hyun-Taek Kim and Hyouk-Bum Kwon for comments on the manuscript, and other members of the Stainier lab for sharing reagents and discussions. This work was supported by postdoctoral fellowships from the Damon Runyon Cancer Research Foundation (DRG#2104-12), Human Frontier Science Program (LT001023/2012-L), and Japan Society for the Promotion of Science to RLM, postdoctoral start-up grants from the Excellence Cluster Cardio Pulmonary System (ECCPS) and German Centre for Cardiovascular Research (DZHK) to RLM, as well as funding from the NIH (HL54737), Packard Foundation and Max Planck Society to DYRS.
Animal experimentation: This study was performed in strict accordance with institutional (UCSF and MPG) and national ethical and animal welfare guidelines. All of the animals were handled according to approved institutional animal care and protocol (Permission No. B2/1068).
- Marianne Bronner, Reviewing Editor, California Institute of Technology, United States
© 2016, Matsuoka et al.
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.