1. Developmental Biology
  2. Neuroscience

Venous endothelin modulates responsiveness of cardiac sympathetic axons to arterial semaphorin

  1. Denise M Poltavski
  2. Pauline Colombier
  3. Jianxin Hu
  4. Alicia Duron
  5. Brian L Black
  6. Takako Makita  Is a corresponding author
  1. Children’s Hospital Los Angeles, University of Southern California Keck School of Medicine, United States
  2. University of California, San Francisco, United States
  3. Medical University of South Carolina, United States
https://doi.org/10.7554/eLife.42528
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  1. Denise M Poltavski
  2. Pauline Colombier
  3. Jianxin Hu
  4. Alicia Duron
  5. Brian L Black
  6. Takako Makita
(2019)
Venous endothelin modulates responsiveness of cardiac sympathetic axons to arterial semaphorin
eLife 8:e42528.
https://doi.org/10.7554/eLife.42528
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Abstract

Developing neurons of the peripheral nervous system reach their targets via cues that support directional growth, a process known as axon guidance. In investigating how sympathetic axons reach the heart in mice, we discovered that a combination of guidance cues are employed in sequence to refine axon outgrowth, a process we term second-order guidance. Specifically, endothelin-1 induces sympathetic neurons expressing the receptor Ednra to project to the vena cavae leading to the heart. Endothelin signaling in turn induces expression of the repulsive receptor Plexin-A4, via induction of the transcription factor MEF2C. In the absence of endothelin or plexin signaling, sympathetic neurons misproject to incorrect competing vascular trajectories (the dorsal aorta and intercostal arteries). The same anatomical and physiological consequences occur in Ednra+/-; Plxna4+/- double heterozygotes, genetically confirming functional interaction. Second-order axon guidance therefore multiplexes a smaller number of guidance cues in sequential fashion, allowing precise refinement of axon trajectories.

https://doi.org/10.7554/eLife.42528.001

Introduction

The heart is innervated by sympathetic and parasympathetic divisions of the autonomic nervous system, which regulate cardiovascular response to emotion and stress. Normal autonomic function in the heart relies on a proper innervation pattern and establishment of functional synapses by efferent axons from postganglionic autonomic ganglia, which are activated by preganglionic neurons that convey orders from the central nervous system. Postganglionic sympathetic neurons that innervate the heart mostly originate from the cervicothoracic sympathetic ganglia, also called the stellate ganglia (STG). These neurons target the conduction system, cardiomyocytes and coronary vessels of the heart to control heart rate, contractility and myocardial blood flow, respectively. In humans, excess sympathetic input is associated with lethal tachycardia (Cao et al., 2000), whereas decreased sympathetic tone is associated with bradycardia and progressive heart block (Lambert et al., 2010). Although the anatomy and physiology of the cardiac sympathetic system is well-understood, the processes that result in establishment of correct circuitry have been less studied.

During embryonic development, sympathetic axons throughout the body traverse blood vessels to reach their end-organs, a coordinated organization called neurovascular congruence. While sympathetic axons follow arteries in virtually all other cases, we discovered that cardiac sympathetic axons from the STGs are unique in following veins to reach the heart (Manousiouthakis et al., 2014). Specifically, cardiac sympathetic axons from the right STG descend along the right superior vena cava to reach and innervate the sinoatrial (SA) node and the lateral surface of the ventricles, while those from the left STG extend along the left superior vena cava, the left sinus horn, the sinus venosus, and project further onto the dorsal surface of the ventricular chamber. The selection of these venous routes is an elegant developmental solution that reflects the anatomical location of the primary cardiac STG targets, which are positioned adjacent to or closest to veins rather than arteries (e.g., the SA node is located at the junction of the right atrium and the superior vena cava). In contrast, a separate subset of STG axons project to the thoracic body wall, the arms, and the dorsal region of the neck, and these follow arteries (specifically, intercostal, subclavian, and vertebral arteries, respectively) to reach these non-cardiac targets.

One mechanism that underlies neurovascular congruence is the secretion of factors from the blood vessel that serve as guidance or growth and survival factors for axonal extension. In cardiac sympathetic innervation, we previously demonstrated that endothelin-1 (Edn1), which is selectively expressed by the endothelium of the cardiac veins, directs axonal growth towards and along these venous routes by the subset of STG neurons (approx. 50%) that express the endothelin receptor Ednra (Manousiouthakis et al., 2014). In mice, axons from the STG initiate extension toward the heart at embryonic day (E) 14.5 and have reached the heart by E15.5. The functional role of endothelin signaling was demonstrated in Edn1-Ednra signaling deficient mouse embryos, which showed a significant reduction of cardiac sympathetic axons reaching the SA node and the ventricular myocardium at E15.5. This deficiency of sympathetic innervation persisted into the postnatal period, and as a consequence, mutant mice were substantially compromised in ionotropic response to sympathetic activation (i.e., amphetamine-induced increased heart rate). Edn1-Ednra signaling, therefore, is a critical axon guidance mechanism that controls the development and ultimate function of the cardiac sympathetic nervous system. In the larger sense, all sympathetic nerves must select among a plethora of potentially available intermediate vascular targets. It is assumed that the complex circuitry of the sympathetic nervous system reflects the expression of a number of tropic and trophic factors such as Edn1 by different vascular elements, and a diversity of neurons that express the appropriate corresponding receptors for these agents. This framework could explain the selection of specific venous and specific arterial routes by different subsets of STG neurons, although the molecular features that account for this circuitry are still only superficially understood.

In this study, we investigate a further and previously unrecognized feature of Edn1-Ednra signaling in cardiac sympathetic axon guidance. We demonstrate that venous endothelium-derived Edn1 not only instructs Ednra+ sympathetic axon guidance to the heart, but also induces the ability of these axons to repel from competing arterial routes by upregulating the expression of Plexin-A4 in Ednra+ STG neurons. Lacking this second layer of guidance, cardiac sympathetic axons misproject to ectopic targets, and as a result, cardiac sympathetic innervation and physiology are both compromised. This analysis reveals that positive axon guidance alone is insufficient to accomplish correct circuitry, and defines a molecular mechanism by which axon attraction and repulsion are coordinately controlled to synergistically accomplish proper innervation.

Results

Edn1-Ednra signaling deficient STG axons misproject along arteries

In addition to neurons that project via veins to the heart, different subsets of STG neurons follow arteries to supply sympathetic innervation to muscles, glands and blood vessels of the dorsal part of the neck, forelimbs and upper thoracic body wall. Previously, we demonstrated a significant loss of sympathetic axons that follow the superior vena cavae to reach the heart in the absence of Edn1-Ednra signaling (Manousiouthakis et al., 2014). Given the choices of arterial routes in their vicinity, it still remained unclear whether Ednra+ STG axons do not project at all, follow other arterial routes, or project in an atypical manner when they are not properly instructed by venous endothelium-derived Edn1. The vena cavae, descending aorta, aortic arch and ductus arteriosus, and the vertebral, subclavian, and intercostal arteries represent the sum of available vascular routes by which STG neurons can project. To address this question, we used tyrosine hydroxylase (Th) immunostaining to map sympathetic axonal projections from the STG in mouse embryonic upper thoraxes. During cardiac sympathetic axonal extension along the superior vena cavae, the STGs are located at the axial level of the lowest cervical vertebra (C7) and are fused with the upper thoracic sympathetic chain ganglia (Figure 1a). The right STG complex stretches from the bifurcation of the brachiocephalic artery to the third thoracic vertebra. Thus, in addition to the heart (primarily the cardiac conduction system), neck and right forelimbs, the right STG neurons supply the upper right chest wall by extending axons laterally but not medially along the right posterior intercostal arteries, which originate from the descending thoracic aorta. Similarly, the left STG complex, which spreads from a position dorsolateral to the aortic arch to the third thoracic column, also extends axons laterally but not medially along the left posterior intercostal arteries to innervate the left upper chest wall. In the presence of normal Edn1-Ednra cardiac sympathetic axon guidance, very few Th+ axons were found in the dorsal-medial region of the upper thorax (T1-T3 level) (Figure 1i), whereas posterior thoracic sympathetic chain ganglia (T4 and below) actively project both medially to the dorsal aorta and laterally along the intercostal arteries.

Figure 1
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Edn1-Ednra signaling mutant STGs project ectopically.

(a–h) Wholemount Th immunostaining visualizing sympathetic projections from STGs in E15.5 thoraxes (a–d) and hearts (e–h) from Ednra-/- (b, f), Edn1-/- (c, g), Ece1-/- (d, h) and a control (a, e) embryos. Black arrows denote ectopic medial projections from Edn1-Ednra signaling-deficient STGs to the thoracic aorta (b–d), which is associated with reduced cardiac sympathetic innervations (f, g, h) (Manousiouthakis et al., 2014); very rare projections from the STG to the dorsal aorta occur in control embryos (arrow in a). (i) A compiled representation of Th+ area in the medial upper thorax area in E15.5 endothelin signaling component mutant embryos. For the embryos of each litter, the proportion of Th+ pixel area within the upper thoracic body wall area (between C7 and T4 vertebrae) between sympathetic chains was measured. Analysis included results of 5 Ednra litters (7 controls, 10 Ednra-/-), 4 Edn1 litters (9 controls, 9 Edn1-/-), and 7 Ece1 litters (18 controls, 15 Ece1-/-). Error bars; mean ± sd. *p=8.49E-22, **p=8.22E-25, ***p=1.71E-19. (j–q) Serial transverse sections of an E15.5 Ednra-/- embryo at the levels corresponding to the white dotted arrows in (b) (from the top: T2 vertebral body, the second rib, T3 vertebral body, and the third rib) were immunostained for Th (brown) and counterstained with hematoxylin (blue). (n–q) Magnified views of bracketed areas in j–m). Red arrows point to ectopic medial projections from STG that are associated with thoracic arteries. dAo, descending aorta; es, esophagus; LA, left atrium; lsvc, left superior vena cava; LV, left ventricle; pia, posterior intercostal artery; RA, right atrium; rsvc, right superior vena cava; RV, right ventricle; stg, stellate ganglion; sv, sinus venosus; T, thoracic segment; tr, trachea; X, Xth cranial nerve. Scale bars, 200 μm (a–d), 100 μm (e–h), 200 μm (j–m), 100 μm (n–q).

https://doi.org/10.7554/eLife.42528.002

As we previously reported, mouse mutations in genes encoding Edn1-Ednra signaling components (endothelin receptor Ednra, endothelin ligand Edn1, and endothelin converting enzyme Ece1) all resulted in reduced sympathetic innervation of the heart (Manousiouthakis et al., 2014) (Figure 1f–h). We found that Edn1-Ednra signaling-deficient STG complexes also abnormally project medially across the dorsal wall of the thoracic cavity, and ultimately reach the descending aorta (Figure 1b–d and i). Ectopic projections originating throughout the craniocaudal domain of the STG (i.e., C7-T3 level) were evident from both left and right STG complexes. Histological analyses showed that these ectopic projections were associated with the posterior intercostal arteries and the right subclavian artery, which are visceral branches of the thoracic aorta (Figure 1j–q), suggesting that STG axons that either do (Edn1 and Ece1 mutants) or should (Ednra mutants) express Ednra failed to follow their normal venous routes, and instead take nearby, albeit ectopic, arterial routes to reach improper targets. Arteries are known to secrete a number of tropic and trophic factors (Brunet et al., 2014; Enomoto et al., 2001; Francis et al., 1999; Honma et al., 2002; Makita et al., 2008); this behavior underlies the arterial selection by most sympathetic axons throughout the body. The observations above indicate that endothelin signaling is required for cardiac sympathetic axons to choose venous routes to the heart and is also required for those axons to not follow ectopic arterial routes.

Edn1-Ednra signaling deficient STG exhibit reduced repulsive response to arteries in vitro

To further understand the relationship between endothelin signaling and inappropriate STG arterial targets, we explanted STGs in a collagen gel and co-cultured with dissected vascular segments in the absence of any exogenous factors. Without exogenous factors or without coculture with vascular tissue, sympathetic ganglia do not initiate outgrowth. In our previous study, we used this assay to evaluate tropic (attractive) and trophic (growth promoting) effects of venous segments in STG neurite outgrowth and to demonstrate that venous segment-derived Edn1 acts as an attractive factor for Ednra+ STG neurons in vitro (Manousiouthakis et al., 2014). Here, we co-cultured STG explants with thoracic aortic segments, both isolated from embryos at E14.5, a time at which normal STG neurons have already been exposed to venous-derived Edn1. Similar to the response to venous segments, wild-type thoracic aortic segments exhibited a strong attractive effect on wild-type STG neurite outgrowth (Figure 2a and c). However, unlike the response to the venous segments, a large fraction of control neurites in the proximal quadrant either stopped midway to the aortic segment (Figure 2a yellow dot, 2d) or turned away from the aortic segment (Figure 2a red dots, 2d). This is consistent with the presence of chemorepulsive signals originating from the aortic tissue that are received by a subset of STG neurons. Control STGs showed the same behavior when co-cultured with Ednra-/- aortic segments (Figure 2c and d). Ednra-deficient STGs showed initial neurite outgrowth towards aortic segments similar to the controls (Figure 2b and c). Interestingly, however, a much greater fraction of Ednra-deficient neurites grew into or turned towards the aortic segments (Figure 2b blue dots; Figure 2d blue bars), and reciprocally, fewer neurites stopped or turned away from the aortic segment (Figure 2b and d). These observations collectively suggest that, in addition to tropic and trophic factors, the thoracic aorta also expresses factor(s) that are repulsive for a subset of sympathetic axons of the STGs, and furthermore, that Ednra is intrinsically required in these STG neurons to respond to these repulsive guidance cue(s) emanating from the thoracic aorta. The approximately half of control STG neurons that project to the aortic segment (Figure 2d) is presumed to overlap with the approximately half of STG neurons that do not express Ednra (Manousiouthakis et al., 2014), and therefore are nonresponsive to these repulsive cues.

Figure 2
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Lack of repulsive response to arterial segments in Ednra-deficient STGs in vitro.

(a–b) Neurite outgrowths from E14.5 control STG (a) and Ednra-/- STG (b) cocultured with thoracic descending aorta segments (dAo) dissected from littermate control embryos were visualized by wholemount Th immunostaining. Red, yellow and blue dots denote neurites that have turned away from, have stopped extending toward, or have grown into the vascular segment (proximal quadrant), respectively. (c) A compiled representation of directional outgrowth (pixel area in the proximal quadrant) from the STG in terms of relative neurite outgrowth projecting proximally, laterally, or distally to the dAo. For each experiment, total neurite outgrowth from the STG (sum of all four quadrants) was defined as 100%, and neurite outgrowth in each quadrant is shown as a fraction of total outgrowth. (d) A compiled representation of growth tip directions of neurites within the proximal quadrant shown in (c). Total number of growth tips scored in each proximal quadrant was defined as 100%, and the number of growth tips directing away, stopped, or growing toward the co-cultured dAo segments are shown as a fraction of total neurites in the proximal quadrant. (c–d) Analysis includes results of control:control (n = 15), control:Ednra-/- (n = 6), Ednra-/-:control (n = 10) and Th-Cre/Ednra:control (n = 6) pairs from seven different litters. A total of 183 growth tips in the proximal quadrants were scored from the analysis and compiled in d). Error bars; mean ±s.e.m.; *p=1.53E-08, **p=7.67E-08. Scale bar, 50 μm (a–b).

https://doi.org/10.7554/eLife.42528.003

Reduced expression of Plxna4 in endothelin signaling deficient STG neurons

Semaphorin-plexin/neuropilin signaling is known to serve as a repulsive guidance mechanism for developing sympathetic neurons. Plexin-A3 (Plxna3) and Plexin-A4 (Plxna4) are expressed in sympathetic neurons (Cheng et al., 2001), and Plxna4 mutant mice display ectopic medial projections from the sympathetic ganglia (Waimey et al., 2008). Sema3a mutation, and neural crest-specific deletion of Nrp1 (which includes all sympathetic neurons), were also shown to result in ectopic medial projections from the thoracic sympathetic ganglia, coupled with reduced sympathetic innervation of the heart (Ieda et al., 2007; Maden et al., 2012). The apparent similarity of these ectopic projection phenotypes with those that we observed in endothelin mutants suggested the possibility that endothelin signaling might interact with semaphorin signaling to control the repulsive response of STG axons to aortic arterial segments.

To ask if endothelin signaling alters the expression of semaphorin receptors, we isolated STG individually from Ednra-/-, Edn1-/-, Ece1-/- and their littermate control embryos and extracted RNA for real-time PCR analysis of Nrp1, Plxna3, and Plxna4 gene expression (Figure 3a). In all Edn1-Ednra signaling deficient STGs, Plxna4 expression was reduced by half, whereas expression of Nrp1 and Plxna3 was unaffected. Because the Ednra gene is expressed only in a subset (approx. half) of STG neurons (Manousiouthakis et al., 2014), the 50% reduction in Plxna4 expression in Ednra-deficient STG could reflect a complete loss of expression in the Ednra+ population, with the gene still expressed in the other half of STG neurons. To address this possibility, we examined Plexin-A4 protein expression by immunofluorescence detection in histological sections. Indeed, in control embryos, Plexin-A4 was detected in Th+ cardiac sympathetic axons that descended along the superior vena cavae (Figure 3d–e,h–i). In littermate Ednra mutant embryos, there was no detectable level of Plexin-A4 expression in sympathetic axons that misprojected along the thoracic aorta and the intercostal arteries (Figure 3j–k and l–m, yellow arrows), whereas axons associated with the superior vena cavae retained Plexin-A4 expression (Figure 3j–k and l–m, white arrowheads). The former are presumably STG-derived that would normally have projected to the heart; the latter are endothelin-insensitive and presumably represent Ednra-negative subsets of neurons that reach the heart from the STG (as in Figure 1f–h). These results suggest that venous Edn1 is an upstream regulator of Plxna4 gene expression within Ednra+ cardiac STG neurons.

Figure 3
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Reduced expression of Plxna4 in Ednra-deficient STGs.

(a) Quantitative real-time PCR analysis for class three semaphorin receptor and co-receptor genes. Total RNA was extracted from individual E14.5 STG isolated from total seven different litters, reverse transcribed, and evaluated for gene expression as described in Methods. Normalized averaged absolute values for control STGs (n = 15) were scaled at 1.0. Error bars; mean ±s.e.m.; *p=0.002, **p=0.0016, ***p=0.095. (b–m) Serial histological sections of Ednra-/- (c, f–g, j–m) and littermate control (b, d–e, h–i) immunostained for Th (b–c) or immunofluorescence labeled for Th (green) or Plexin-A4 (magenta). Magnified views from an adjacent section of the bracketed areas in b) including the right superior vena cava (rsvc) and left superior vena cava (lsvc) are shown in (d-e and h–i), respectively. Magnified views from an adjacent section of the bracketed areas in (c) including the right superior vena cava (rsvc), left superior vena cava (lsvc), and a posterior intercostal artery (pia) are shown in (f–g), (j–k) and (l-m), respectively. A control pia is not shown because there are no axon misprojections to the pia in normal embryos. White arrowheads point to expression of Plexin-A4 in Th+ cardiac sympathetic axons that are associated with venous routes. Yellow arrows denote lack of Plexin-A4 in Th+ sympathetic axons that are misprojecting along arteries. aAo, ascending aorta; pia, posterior intercostal artery. Scale bars, 200 μm (b–c), 25 μm (d–g), 50 μm (h–k), 50 μm (l–m).

https://doi.org/10.7554/eLife.42528.004

The Plxna4 gene contains an endothelin-induced, MEF2C-dependent transcriptional enhancer

Endothelins regulate gene expression by activation of endothelin-dependent transcription factor binding to conserved elements in several different in vitro and in vivo contexts (Charité et al., 2001; Hu et al., 2015; Kawamura et al., 2004; Sugimoto et al., 2001). We previously demonstrated in vivo that myocyte enhance factor Mef2c gene expression in the neural crest lineage is regulated by endothelin (Hu et al., 2015). Specifically, the Mef2c gene contains an endothelin-dependent MEF2C autoregulatory transcriptional enhancer (Mef2c-F1) element (Hu et al., 2015). Analysis of Mef2c-F1-lacZ transgenic embryos showed that the Mef2c-F1 enhancer is active in sympathetic chain ganglia at E10.5 (Agarwal et al., 2011). Furthermore, E9.5 Mef2c-F1-lacZ embryos cultured in the presence of Edn1 peptide exhibited robust induction of β-galactosidase activity within trunk neural crest cell derivatives (Hu et al., 2015). These observations collectively imply that MEF2C in developing sympathetic neurons could regulate Plxna4 expression in response to endothelin signaling. To further understand how MEF2C might regulate Plxna4 expression in response to endothelin signaling activation, we analyzed MEF2 binding peaks from cortical neurons from a previously published MEF2 ChIP-seq dataset (Telese et al., 2015), and we also assessed evolutionary conservation between mouse, human, and opossum in the Plxna4 locus using the VISTA enhancer browser (Frazer et al., 2004). Using these two complementary approaches, we found a highly conserved MEF2 binding site ~50 kb upstream of the transcription start site (TSS) and four highly conserved MEF2 binding sites located in the third intron of Plxna4 gene (Figure 4a). Each of these five MEF2 sites corresponded to regions identified in ChIP-seq as bona fide sites of MEF2C binding (Telese et al., 2015).

Figure 4
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The Plxna4 locus contains several bona fide, conserved MEF2C sites and expression is induced by endothelin signaling in a MEF2C-dependent manner.

(a) Schematic diagram of conserved MEF2C binding sites in the Plxna4 locus. The Plxna4 locus is shown in the center with transcriptional start site (TSS, bent arrow) and exons (vertical black lines) shown. The track shown above the locus schematic represents a genome browser view of MEF2C binding peaks in the Plxna4 locus obtained from MEF2 ChIP-seq in E15.5 mouse neurons. The red (upstream) and orange (intronic) peaks shown below the locus schematic represent VISTA browser tracks of evolutionary conserved regions in the Plxna4 locus containing conserved MEF2 binding sites in mouse, human, and opossum. rVista alignment of mouse and human genomic sequences showing a detailed view of the MEF2 binding sequences are indicated below. (b) Relative endothelin-dependent induction of Plxna4 gene expression in neural crest cells sorted and isolated from Mef2c-deficient and control embryo explants treated with Edn1 and measured by RNA-sequencing. Error bars; mean ± s.d.. (c–d) Wholemount Th immunostaining visualizing sympathetic projections from STG in E15.5 thoraxes from Mef2cKO (d) and a littermate control (c) embryos. Black arrows denote ectopic medial projections from Mef2C-deficient STGs to the thoracic aorta (d). (e–f) Serial histological sections of Mef2cNCKO mutant embryo (f, i–l) and littermate control (e, g–h) immunostained for Th (e–f) or immunofluorescence labeled for Th (green) or Plexin-A4 (magenta) (g–l). Magnified view from an adjacent section of the bracketed areas in (e) including the left superior vena cava (lsvc) is shown in (g–h). Magnified views from an adjacent section of the bracketed areas in (f) including the left superior vena cava (lsvc), and an aortic arch (AA) are shown in (i–j) and (k–l), respectively. White arrowheads point to expression of Plexin-A4 in Th+ cardiac sympathetic axons that are associated with venous routes. Yellow arrows denote lack of Plexin-A4 in Th+ sympathetic axons that are associated with arteries. Scale bars, 200 μm (c–d, e–f), 50 μm (g–l).

https://doi.org/10.7554/eLife.42528.005

To test whether the Plxna4 gene was responsive to endothelin signaling via MEF2C, we analyzed RNA expression in FACS sorted neural crest cells purified from Mef2c neural crest-specific knockout (Mef2cflox/-; Wnt1a-Cre) [Mef2cNCKO] and littermate control embryos cultured in the presence or absence of exogenous Edn1. To minimize detection of endothelin-independent induction of Plxna4 gene expression, we treated explanted E9.5 embryos, a time at which Plxna4 is not yet actively expressed in sympathetic progenitor cells. Importantly, we observed robust upregulation of Plxna4 gene expression in Edn1-treated control neural crest-derived cells (Figure 4b). In the absence of Mef2c function in the neural crest, Edn1 induction of Plxna4 expression was significantly attenuated compared to Edn1 induction of Plxna4 expression in control neural crest (Figure 4b), supporting the notion that Plxna4 is a MEF2C target in response to endothelin signaling.

If MEF2C mediates Plxna4 expression in an endothelin-dependent manner in vivo, a prediction is that absence of Mef2c should results in misprojection of cardiac sympathetic axons from the STG, as seen in Plxna4 (Waimey et al., 2008) and Edn-Ednra signaling component mutant embryos (Figure 1b–d). To address this, we used wholemount Th visualization of thoracic sympathetic axons in E15.5 Mef2c-deficient embryos. Indeed, we observed ectopic medial projections from the STG (including T1 through T3 sympathetic chain segments) towards the dorsal aorta in Mef2c mutant embryos (Figure 4c–d). This misprojection phenotype is strikingly comparable to that observed in Edn1-Ednra signaling component deficient embryos (Figure 1b–d). We also evaluated the expression of Plexin-A4 in different subsets of sympathetic axons in control and Mef2cNCKO mutant embryos (Figure 4e–l). Just as observed in Ednra mutants (Figure 3b–m), axons associated with the superior vena cavae retained Plexin-A4 expression in Mef2cNCKO mutant embryos (Figure 4f and i–j). In contrast, sympathetic axons associated with the thoracic aorta did not express Plexin-A4 in Mef2cNCKO mutant embryos (Figure 4f and k–l), which we also observed in Ednra mutants (Figure 3c,j–m). Taken together, these observations are consistent with the interpretation that in the endothelin-dependent subset of cardiac sympathetic axons, Edn1 induces Plxna4 expression via MEF2C to support proper axon guidance, whereas endothelin-independent subsets of STG axons express Plxna4 in a MEF2C-independent manner.

Genetic relationship between Ednra and Plxna4 in cardiac sympathetic axon guidance

To further determine if the Ednra and Plxna4 genes are functionally related in cardiac sympathetic axon guidance, we took a genetic approach that involved analysis of postnatal mice that were heterozygous at the Ednra and Plxna4 loci. A phenotypic consequence in double heterozygotes when each single heterozygote is normal suggests that the two genes might be functionally related or function in a common pathway. In any case, a genetic interaction observed in compound heterozygotes suggests that lowering the expression of both gene product together reduces downstream signaling below a threshold level where a phenotype emerges.

As we described previously (Manousiouthakis et al., 2014), the extent of sympathetic innervation of the heart is compromised in Th-Cre; Ednrafl/- conditional null mice (Figure 5d, Figure 5—figure supplement 1a). We observed a similar degree of impairment in sympathetic-neuron-specific Th-Cre; Ednrafl/+; Plxna4+/- double heterozygous mice (Figure 5c, Figure 5—figure supplement 1a–b). In sections through the SA node, using HCN4 as a marker of conduction system cardiomyocytes, Th+ nerve fibers were obviously reduced in number and caliber, although still present, in double heterozygous hearts (Figure 5k, Figure 5—figure supplement 1b). We used synaptophysin (Syp), which is expressed in presynaptic sites, to determine if active synapses were formed by these nerve endings. The level of Syp staining was reduced commensurate with the reduction of Th staining (Figure 5l–m, Figure 5—figure supplement 1b), although not altered in a manner that would suggest an independent defect in synapse formation. A similar deficiency in sympathetic axon density and presynaptic assembly was evident in the ventricular myocardium (Figure 5u–v). Because these residual nerves are present at similar levels in both double heterozygous and conditional Ednra-null hearts (Figure 5n–p and w–x, Figure 5—figure supplement 1a–b), we interpret these to be a separate subset of sympathetic nerves that reach the heart in an endothelin signaling-independent manner.

Figure 5 with 1 supplement see all
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Ednra and Plxna4 interact genetically.

(a–d) Wholemount immunostaining visualizing the dorsal surface of hearts from a 7-week-old Th-Cre; Ednrafl/+; Plxna4+/- double heterozygote (c), a Th-Cre; Ednrafl/- mutant (d), and single heterozygote controls Th-Cre; Ednrafl/+ (a) and Plxna4+/- (b). a littermate control (a). (e–x) 300 μm vibratome sections immunofluorescence labeled for HCN4 (cyan), Th (magenta) and SYP (yellow) visualizing sympathetic presynaptic morphologies in the SA node (e–p) and left ventricular myocardium (q–x) of an adult mice. ca, coronary (circumflex) artery, ivc, inferior vena cava. Scale bars, 500 μm (a–d), 50 μm (e–x).

https://doi.org/10.7554/eLife.42528.006

To more rigorously examine the endothelin-plexin genetic interaction and its functional consequences, we undertook electrocardiography (ECG) analysis. As described previously (Manousiouthakis et al., 2014), amphetamine treatment acutely induces noradrenaline release at sympathetic termini. In turn, noradrenalin activates beta-adrenergic receptors in the cardiac conduction system and the resulting increase in heart rate is a quantitative measure of cardiac sympathetic nerve density and functionality. Mice heterozygous at the Ednra or Plxna4 loci individually responded normally to amphetamine in the acute period (<2 min after injection) by increasing heart rate (Figure 6a), which indicates that sympathetic innervation and functionality are insensitive to loss of one copy of either Ednra or Plxna4. However, Ednra; Plxna4 double heterozygous mice (Ednra+/-; Plxna4+/-) and conditional Ednra-Plxna4 double-heterozygous mice (Th-Cre; Ednrafl/+; Plxna4+/-) exhibited a severely blunted acute ionotropic response, nearing the completely eliminated response of homozygous sympathetic-neuron-specific Ednra mutants (Th-Cre; Ednrafl/-) (Figure 6a). These observations support the interpretation that the Ednra and Plxna4 genes are coupled in cardiac sympathetic axon guidance in a physiologically relevant manner. Amphetamine eventually induces noradrenaline and adrenaline release from the brain and adrenal glands, respectively, which ultimately influence heart rate through systemic circulation. This delayed response (monitored 10 min after injection) was fully intact in all double-heterozygous mice (Figure 6b), which demonstrates that the noradrenergic and adrenergic systems in the central nervous system and adrenal glands are intact in double heterozygous mice. Furthermore, these mice were normally responsive to the beta-adrenergic receptor agonist isoproterenol (Figure 6c), indicating that the cardiomyocyte-specific components of the conduction system and myocardium that respond to sympathetic inputs are functional in the double-heterozygous background.

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Ednra-Plxna4 double-heterozygous mice exhibit diminished cardiac sympathetic nerve activity.

(a–c) Changes in heart rate following amphetamine (a;<2 min, (b;>10 min) and isoproterenol (c) administration measured in indicated 7-week-old single heterozygotes, double heterozygotes, conditional Ednra mutants, and their littermate wildtype controls. Error bars; mean ± s.e.m.; *p=8.95E-05, **p=4.88E-04, ***p=2.55E-05. (d) A compiled representation of the low-frequency: high-frequency domain (LF/HF) ratio at the baseline, post-amphetamine and post-isoproterenol administration in mice of the indicated genotypes. Frequency-domain was extracted from power spectral analysis of heart rate variability (HRV) shown in Figure 6—figure supplement 1. Error bars; mean ± s.e.m.; *p=0.0001, **p=0.0002, ***p=1.02E-06, †p=0.03, ††p=0.077, †††p=8.39E-05. NS, not significant.

https://doi.org/10.7554/eLife.42528.008

Sympathetic versus parasympathetic activities can also be evaluated by heart rate variability (HRV) (Akselrod et al., 1981). HRV represents physiological rhythm fluctuations between consecutive beats: beat-to-beat fluctuation is minimal in the resting state, whereas in the conscious state, the interval between consecutive beats becomes more variable because of fluctuations in the opposing actions of sympathetic and parasympathetic inputs. HRV is divided into low-frequency (LF) and high-frequency (HF) components, and commonly described by the LF/HF ratio (Figure 6d). In Th-Cre; Ednrafl/- mutants, in which sympathetic innervation and activity are reduced (Figure 5d, n–p and w–x), a significant reduction of the LF component was observed (Figure 6d, Figure 6—figure supplement 1c), which indicates less cardiac sympathetic neural activity in the baseline state. Th-Cre; Ednrafl/+; Plxna4+/- ± also exhibited a similar reduction of the LF/HF ratio (Figure 6d, Figure 6—figure supplement 1b), coinciding with their reduced cardiac sympathetic innervation (Figure 5c, k–m and u–v). Single heterozygote mice for either Ednra or Plxna4 were unaffected (Figure 6d). Amphetamine treatment increases the LF/HF ratio in normal mice by activating sympathetic activity, but this did not change in the compound mutants, which coincides with their attenuated change in heart rate after acute amphetamine treatment (Figure 6d). Similarly, isoproterenol treatment increased the LF/HF ratio in all mice (Figure 6d). These observations collectively demonstrate that endothelin control of Plxna4 expression is intrinsically required for Ednra+ STG neurons to follow venous routes to reach the heart, and that this subset of STG neurons is required for normal cardiac sympathetic function.

Endothelin signaling is also required for a subset of axons from the superior cervical ganglia (SCG) to properly project along the external carotid arteries to targets in the head and neck (other neurons project along the internal carotid arteries in an endothelin-independent manner to reach different targets in the head) (Makita et al., 2008). This system relies on spatial and temporal expression of the ligand Edn3 by smooth muscle cells of the 3rd pharyngeal arch arteries during the E11.5–12.5 period, which is in contrast to expression of Edn1 by endothelium of the vena cavae at E14.5 and onward for STG projections to the heart. Despite the utilization of these two different ligands, the SCG and STG both employ the same endothelin receptor, Ednra, for guidance. Plxna4 mutants show an SCG misprojection phenotype (Waimey et al., 2008) that results in fewer SCG axons extending along the external carotid arteries (Figure 7c and g). Because of these observations, we histologically analyzed E14.5 Ednra+/-; Plxna4+/- ± heterozygote embryos for evidence of genetic interaction of the Ednra and Plxna4 genes in SCG axon guidance. Interestingly, however, Ednra-Plxna4 double heterozygotes were unaffected in SCG external carotid artery projection (Figure 7b and f). This indicates that Ednra-Plxna4 interaction is not a general phenomenon for all sympathetic axon guidance, but rather is specific for the cardiac sympathetic axons from the STG. One possible explanation for this observation is that the Plxna4 and Ednra mutant SCG phenotypes are superficially similar but are not identical: absence of Plxna4 results in randomized outgrowth (Figure 7c, red arrows), whereas absence of Ednra eliminates guidance towards the external carotid arteries (Figure 7d). Consequently, in SCG axon outgrowth, Ednra and Plxna4 may have different roles that do not synergize in Ednra+/-;Plxna4+/- ± heterozygotes. In contrast, the STG projection and cardiac innervation phenotypes of Ednra mutants, Plxna4 mutants, and Ednra+/-;Plxna4+/- ± heterozygotes are all seemingly identical (Figure 1, Figure 5).

Figure 7
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Normal SCG axonal projections along the external carotid arteries in Ednra-Plxna4 trans-heterozygotes.

(a–h) Transverse sections from E14.5 Ednra+/-; Plxna4+/- (b, f), Plxna4-/- (c, g), Ednra-/- (d, h) mutant embryos and a littermate control embryo at the level of carotid artery bifurcation (a–d) and the upper larynx (e–h) stained with Th showing sympathetic axons from the SCG extending along the external carotid artery in the trans heterozygote. Black arrows point to normal projections of SCG axons along the external carotid arteries (e, f). Red arrows indicate ectopic (random) sprouts from the SCG in Plxna4-/- mutant embryo (c). Arrowheads denote reduced or defective SCG projections along the external carotid arteries (d, g–h). eca, external carotid artery; ica, internal carotid artery; scg, superior cervical ganglion. Scale bar, 100 μm (a–h).

https://doi.org/10.7554/eLife.42528.010

Ednra deficient STG fail to repel arterial semaphorin in vitro

The activation of class A plexins (with co-receptor neuropilins) requires interaction with secreted class three semaphorins (Janssen et al., 2012). Among class three semaphorins, Sema3a and Sema3f serve as ligands for Plexin-A4 in various biological contexts (Suto et al., 2005; Yaron et al., 2005). Sema3a and Sema3f are both expressed by the dermomyotome, forelimbs and paraxial mesoderm during the E10.5–12.5 period (Kawasaki et al., 2002; Maden et al., 2012), and Sema3a and Sema3f mutant embryos independently display medial ectopic projections from sympathetic ganglia in the upper thorax (Maden et al., 2012). We confirmed selective expression of Sema3a and Sema3f in the smooth muscle layer of the upper thoracic aorta during the critical period of cardiac sympathetic axonal extension to the heart (Figure 8—figure supplement 1a–d and e–h). To test the hypothesis that arterial semaphorin(s) repel STG axons in an Edn1-Ednra-dependent manner, we next used in vitro STG explant culture with COS cell aggregates. As noted above, in minimal growth medium with no growth/trophic factors added, STG isolated from E14.5 control embryos and explanted alone do not extend neurites (Manousiouthakis et al., 2014). Regardless of Ednra or Plxna4 genotype, STG exhibited a robust tropic and trophic response to aggregates of untransfected COS cells, indicating that COS cells secrete factors (which are not defined) that are active on sympathetic neurons (Figure 8a–d). When control STGs were placed between untransfected and Sema3a-transfected COS cell aggregates (GFP+) (Figure 8i), neurites only projected away from the Sema3a-expressing cells (Figure 8e and j), demonstrating the repulsive nature of Sema3a signaling on all STG sympathetic axons (all of which, including Ednra+ neurites in control STGs, express Plexins). Neurites from Ednra+/- or Plxna4+/- STGs showed a similar response to Sema3a-expressing COS aggregates as control STGs (Figure 8j). In contrast, however, Ednra-deficient STGs exhibited a fraction of neurite outgrowth that was attracted towards the Sema3a-expressing COS aggregate (Figure 8g and j). A similar response was observed in Ednra-Plxna4 double heterozygote STG and Plxna4-null-STG explants (Figure 8f, h and j). As described above, Ednra is expressed only by half of STG neurons while Plxna4 is expressed in most STG neurons.

Figure 8 with 1 supplement see all
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Ednra-deficient STGs show reduced repulsive response to Sema3a in vitro.

(a–h) Neurite outgrowth from explanted STG co-cultured with COS cell aggregates were visualized by whole mount Th staining. STG dissected from E14.5 embryos of the genotypes indicated at left were cultured in the proximity of untransfected-COS cell aggregates (a–d) or in between untransfected and Ad-GFP-2A-mSema3a- transfected-COS cell aggregates (e–h). Sema3a expression of transfected-COS cell aggregates are confirmed by GFP expression (green; e–h). The repulsive effect was measured by neurite outgrowth length towards the untransfected-COS aggregate as positive numbers and towards Sema3a-transfected-COS aggregates as negative numbers, as indicated in (i). To control for experimental variation, the distance between the STG and the COS aggregates (d1) was defined as 1.0 or −1.0 and each neurite outgrowth length toward either COS aggregate (d2) was normalized as a relative value (d). (j) A compiled dot-whisker plot representation of the repulsive response of STG to Sema3a. Each dot represents the averaged neurite outgrowth from each STG towards untransfected-COS (grey dots) or Sema3a-transfected-COS (green dots) aggregates in each experimental culture. The number of experimental replicates for each STG genotype is as indicated, and analysis includes the total counts of 98 wildtype, 31 Ednra+/-, 24 Plxna4+/-, 91 Ednra+/-; Plxna4+/-, 102 Ednra-/-, 57 Th-Cre/Ednra and 51 Plxna4-/- STG neurites. *p=5.93E-08, **p=7.12E-10, ***p=3.48E-08, ****p=4.97E-07.

https://doi.org/10.7554/eLife.42528.011

Discussion

The complexity of the nervous system is vast. Sympathetic nerves have partially solved the problem of how to reach appropriate targets by restricting their extensions to lie along blood vessels. However, even with this limitation, these nerves must select from among a number of arteries, and as now recognized, also veins, that lie in their vicinity. Selectivity is presumed to be accomplished by expression of a variety of guidance cues by different vascular elements and by expression of a variety of receptors by different subsets of sympathetic neurons. Only a relatively small number of attractive or repulsive guidance cues are known and are too few to explain the complexity of the sympathetic system at least according to a first-order (one-to-one) relationship between guidance cue and guided nerve. One possibility is that many more guidance factors exist but have not yet been discovered. Instead, our study reveals a second order of regulation, in which detection of a first signal (endothelin) by the Ednra+ subset of STG neurons induces expression of a second axon guidance receptor (Plexin-A4) that further refines the selection of vascular targets (Figure 9). Second-order guidance allows a smaller number of guidance cues to be deployed combinatorially to support proper peripheral innervation. This novel feature of axon guidance, which we have studied in the heart, might be more generalizable to other aspects of the peripheral nervous system.

Figure 9
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A model of second-order axon guidance for cardiac sympathetic axons.

An Ednra-expressing STG neuron located in the vicinity of distinct vascular trajectories (vein and artery) sees venous-derived endothelin as a primary attractive guidance cue and initiates axonal extension toward the vein (First Order). Endothelin (Edn1-Ednra) signaling induces MEF2C transcription factor binding to MEF2C response element(s) in the Plxna4 gene promoter to upregulate expression of Plxna4 gene in venous-associated Ednra+ STG neurons. Plexin-A4 then serves as a repulsive guidance receptor for arterial Sema3a (Second Order), which further restricts endothelin-dependent axonal extension along the venous routes by keeping Ednra+ axons from being attracted toward arterial trajectories.

https://doi.org/10.7554/eLife.42528.013

Our results demonstrate that second-order guidance for cardiac sympathetic axons involves Sema3-Plexin-A4 signaling. Arterial selective expression of secreted class three semaphorins (Figure 8—figure supplement 1a–d and e–h), phenotypic (neuroanatomical and physiological) similarities between Edn1-Ednra signaling mutants and Sema3a-Plexin-A4 signaling mutants, and observations from STG explant neurite outgrowth assays collectively support this model. Plexin-A4 can also be directly activated by membrane-bound class six semaphorins (Janssen et al., 2010; Suto et al., 2005; Suto et al., 2007). We detected Sema6a expression in arterial smooth muscle during the critical time period for cardiac sympathetic axonal projections along vascular routes (Figure 8—figure supplement 1i–l). Sema6a expression was also detected within cardiac sympathetic neurons and axons, whereas Sema6b was not expressed in neurons or vasculature (Figure 8—figure supplement 1i–l and m–p). Unlike Sema3a, there is no prior indication that Sema6a mutation results in a cardiac sympathetic phenotype, although we have not yet firmly ruled out if Sema6a influences endothelin-dependent repulsive guidance via Plexin-A4.

The importance of Plexin-A4 as a receptor for Sema3 signals in second order guidance of cardiac sympathetic axons is strongly implicated by the misprojection phenotype of Plxna4 mutants (Waimey et al., 2008) and of Ednra-Plxna4 double heterozygotes (this study). Although mutation of Plxna3 alone does not result in this phenotype, the Plxna3 and Plxna4 double mutant was more severely affected (more ectopic thoracic projections) than Plxna4 single mutants, implying the possibility of functional redundancy. Plexin mediation of class three semaphorin signaling is thought to require the coreceptor neuropilin, and Nrp1 mutation also results in severe ectopic medial projections from the sympathetic ganglia (Kawasaki et al., 2002). It should be noted that Sema3a-Nrp1 signaling also controls sympathetic progenitor cell migration and then the caudal extension of post-migratory sympathetic neurons during the E9.5-E11.5 period (Kawasaki et al., 2002). Thus, ectopic projection phenotypes in these various Sema-Plexin-Nrp mutant backgrounds might be the additive effects of early migration defects coupled with subsequent axon guidance defects. However, Plxna4 mutants are not compromised in early migration or ganglion extension, and only first show a misprojection phenotype at the time of initial axon extension (Waimey et al., 2008).

Our previous (Manousiouthakis et al., 2014) and current studies revealed that STG neurons are heterogeneous: there is an Ednra-expressing subset that extends along venous routes to the heart, an Ednra-negative subset that also extends along venous routes to the heart, and an Ednra-negative subset that extends along arterial routes to innervate the neck, limbs, and thoracic body wall. We propose that the Edn1-MEF2C-Plexin-A4 hierarchy described here serves as a basis of second-order axon guidance that controls cardiac sympathetic innervation for the Ednra-expressing subset of STG neurons. We identified Plxna4 as a downstream target of endothelin signaling, and demonstrated that MEF2C is an endothelin-induced transcription factor that regulates Plxna4 gene expression in developing neural crest cells. Despite its uniform expression in developing sympathetic neurons (Cheng et al., 2001), Plxna4 gene regulation does not require endothelin-dependent MEF2C transactivation in the Ednra-negative subsets of STG neurons, indicating that Plxna4 expression is controlled by other gene regulatory mechanism in those sympathetic neurons.

While second-order guidance is sufficient to explain the major component of STG-cardiac circuitry, several further intriguing questions remain. First, an Ednra-negative subset of STG neurons extends along arterial routes. These neurons express Plexin-A4, which might be expected to cause them to avoid their arterial targets. In fact, in a permissive environment as in our collagen explant assay system, all neurites from control STG exhibit strong repulsive response towards Sema3a-overexpressing COS aggregates (Figure 8). Presumably, in the in vivo environment, additional mechanisms emanating from arteries override Sema3a-Plexin-A4 signaling. These mechanisms may act as stronger attractive cue(s) for sympathetic axons to cancel the repulsive effects on Semaphorin, or may alter expression and/or post-translational modification of Plexin-A4/Npn receptor signaling components to make arterially-committed axons be non-responsive to arterial Semaphorin. If the latter mechanism exists, this would also be considered as an example of second-order axon guidance. Second, while endothelin signaling is needed for the major subset of cardiac sympathetic nerves to express Plexin-A4 and to avoid arterial targets to reach the heart, some level of cardiac sympathetic innervation from the STG still occurs in endothelin signaling mutants (e.g., Figure 1f–h, Figure 5c–d). These neurons are repelled from arteries, in a Plexin-A4-dependent, endothelin-independent manner, but these nerves still follow the vena cavae and reach and innervate the SA node and other cardiac targets. These neurons are either responsive to alternative positive, unidentified guidance cues (other than endothelin) that originate in the vena cavae, or simply follow the vena cavae as a neutral default vascular pathway. The presence of these neurons is not sufficient to facilitate a response to amphetamine, suggesting that they might be functionally distinct from the endothelin-dependent subset; alternatively, there may simply be too few of these neurons to have a functional consequence in this specific physiological process. The role of this subset of neurons in heart biology remains unknown.

Materials and methods

Key resources table
Reagent type (species) or resourceDesignationSource or referenceIdentifiersAdditional information
Genetic reagent
(M. musculus)		Ednrafl, ETAfloxPMID: 14585980MGI:2687362,
RRID:IMSR_RBRC06323
Genetic reagent
(M. musculus)		MEF2Cfl, Mef2cloxPPMID: 17336904MGI:3718323
Genetic reagent
(M. musculus)		Edn1-, EdnRA-, ET-1-PMID: 8152482MGI:1857637
Genetic reagent
(M. musculus)		Ece1-, ECE-1 -PMID: 9449665MGI:2158947,
RRID:IMSR_RBRC06166
Genetic reagent
(M. musculus)		Plxna4-, PLA4 KO,
PlexinA4-		PMID: 15721238MGI:3579185,
RRID:MMRRC_030407-MU
Genetic reagent
(M. musculus)		ThCre, Th::CrePMID: 1785595MGI:5607431,
RRID:MMRRC_029177-UCD
Genetic reagent
(M. musculus)		Wnt1Cre,
Tg(Wnt1-cre/Esr1)10Rth		PMID: 9843687MGI:2447684
Cell line
(Cercopithecus aethiops)		COS-7ATCCCRL-1651,
RRID: CVCL_0224		LOT: 5784927
Originally tested
negative for Mycoplasma,
Bacterial and fungal
contamination (purchase date:6/30/2016).
Cells have not independently
authenticated for each passage used
for experiments and data collection.
Cells were not independently
tested for mycoplasma contamination.
AntibodySheep polyclonal
anti-Tyrosine
Hydroxylase		MilliporeAB1542,
RRID:AB_90755		IHC (1:400)
AntibodyRabbit polyclonal
anti-Plexin A4		Novus BiologicalMBP1-85128,
RRID:AB_11013411		IHC (1:400)
AntibodyRabbit polyclonal
anti-Semaphorin 3A		Abcamab23393,
RRID: AB_447408		IHC (1:300)
AntibodyRabbit polyclonal
anti-Semaphorin 3F		Abcaman203394,
RRID:AB_2783521		IHC (1:500)
AntibodyRabbit polyclonal
anti-Semaphorin 6A		Abcamab72369IHC (1:200)
AntibodyMouse monoclonal
anti-Semaphorin 6B		SCBTsc-390928,
RRID:AB_2783522		IHC (1:200)
AntibodyRabbit polyclonal
anti-HCN4		Abcamab69054,
RRID: AB_1861080		IHC (1:500)
AntibodyMouse monoclonal
anti-SYP		SCBTsc-17750,
RRID: AB_628311		IHC (1:500)
Recombinant
DNA reagent		Ad-GFP-2A-mSema3AVectorBioADV-271580
Sequence-based
reagent		qRT-PCR primers (hprt)primer bank
ID: 7305155a1
Sequence-based
reagent		qRT-PCR primers (nrp1)primer bank
ID: 6679134a1
Sequence-based
reagent		qRT-PCR primers (plxna3)primer bank
ID: 667939a1
Sequence-based
reagent		qRT-PCR primers (plxna4)primer bank
ID: 28461143a1
Commercial
assay or kit		RNaseOUTThermofisher10777019
Commercial
assay or kit		Trizol LSThermofisher10296028
Commercial
assay or kit		RNeasy Micro KitQiagen74004
Commercial
assay or kit		Ovation RNA-Seq
System V2		NuGEN
Commercial
assay or kit		Encore Rapid
Library System		NuGEN
Chemical
compound, drug		amphetamineSigma A5880
Chemical
compound, drug		isoproterenolSigma I6504
Chemical
compound, drug		propranololSigma P0884
Software, algorithmFiji - Image Jhttps://imagej.net/FijiRRID:SCR_003070
Software, algorithmCASAVA (v1.8.2)IlluminaRRID:SCR_001802
Software, algorithmtophat v1.3Trapnell et al. (2009)doi:10.1093/
bioinformatics/btp120
Software, algorithmU-Seq version
8.0.2		Nix et al. (2008)doi:10.1186/1471
-2105-9-523
Software, algorithmLabChart 8AD InstrumentsRRID:SCR_001620

Animals

The Th-Cre (Gong et al., 2007), Wnt1-Cre (Danielian et al., 1998), Ednra (Clouthier et al., 1998), Edn1 (Kurihara et al., 1995), Ece1 (Yanagisawa et al., 1998), Plxna4 (Yaron et al., 2005) (MMRRC U420D020918), conditional Ednra (Kedzierski et al., 2003), and conditional Mef2c (Arnold et al., 2007) alleles have been described previously. All experiments with animals complied with National Institute of Health guidelines and were reviewed and approved by the CHLA (274-18), UCSF (AN171342) or MUSC (2018–00627) Institutional Animal Care and Use Committee.

Wholemount Th immunostaining

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Mouse embryo thoraxes were dissected from PFA fixed embryos, dehydrated through a methanol series (50–100%), and incubated overnight in 3%H2O2/20%DMSO/methanol solution to quench endogenous peroxidase activity. Tissues were rehydrated through a methanol series (100–50%) to PBST (1% Tween-20 in PBS), and incubated with sheep anti-Th antibody (1:400; Millipore) for 3 days at 4°C, followed by HRP-conjugated secondary antibody for 3 days at 4°C. Immunoreactive signal was visualized by DAB detection. Tissues were then dehydrated through a methanol series and cleared with benzyl benzoate/benzyl alcohol (2:1). Postnatal hearts were dissected from animals fixed with 4% PFA in PBS by retroaortic perfusion through the dorsal aorta, and then processed for immunostaining as described above. To quantify Th+ axons in the embryonic thoraxes and postnatal hearts, the Th labeled area (binary threshold selection) and the total region of interest (dorsal body wall of the thorax or dorsal surface of the heart) pixel area were measured using Fiji-Image J software.

Immunohistochemistry and immunofluorescence

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PFA fixed embryos were dehydrated, cleared and embedded in paraffin. 10 µm paraffin sections were dewaxed, rehydrated in ethanol series (100–70%) to H2O. Following antigen retrieval by heating in citrate buffer (0.1 M sodium citrate, pH6.0), sections were immunolabeled with anti-Th (1:400; Millipore AB1542), anti-Plexin-A4 (1:400; Novus NBP 1–85128), anti-Sema3a (1:300; Abcam ab23393), anti-Sema3f (1:500; Abcam ab203394), anti-Sema6a (1:200; Abcam ab72369) or anti-Sema6b (1:200; SCBT sc-390928) antibodies. For immunohistochemistry, sections were then incubated with HRP-conjugated secondary antibodies (1:200). Immunoreactive signal was visualized by DAB detection system followed by counterstaining with hematoxylin. For immunofluorescence labeling, histological sections were treated with 0.03% Sudan Black to quench autofluorescence prior to primary antibody incubation. Immunoreactive signals were visualized using Alexa Fluor-conjugated secondary antibodies (Life Science) and counterstained with DAPI. Plexin-A4 immunoreactive signal was visualized with biotin-streptavidin amplification.

For postnatal hearts, 300 μm thick vibratome sections were prepared for immunofluorescence staining. Sections were immunolabeled with anti-HCN4 (1:500; Abcam ab69054), anti-Th (1:400: Millipore AB1542) and anti-SYP (1:500; SCBT sc-17750) antibodies overnight at 37°C, and followed by Alexa Fluor-conjugated secondary antibodies (Life Science) for 3 hr at 37°C. Immunolabeled sections were counterstained with DAPI, cleared with ScaleU2 and flat-mount to histology slides for confocal microscope image acquisition. To quantify SYP+ area in Th+ axons that innervate the SA node, the HCN4+ pixel area was measured, and the SYP+ and Th+ areas were measured by binary threshold selection using Fiji-Image J software.

Embryo explant culture, Edn1-treatment, and RNA-sequencing

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Embryos were explanted at E9.5, and cultured as described previously (Rojas et al., 2005). Explants were cultured for 1 hr prior to treatment with 10 µM Edn1 or vehicle for 24 hr. Following treatment, three explants were pooled for each sample and digested in 300 µl 0.25% trypsin, 0.7 mM EDTA in PBS for 30 min at 37°C. A single cell suspension was formed and 30 µl fetal bovine serum, 10 µl 1M HEPES [pH7.4], and 10 µl RNase inhibitor (RNaseOUT, Invitrogen) were added. Cells were FACS sorted into 500 µl of Trizol LS (Invitrogen) and RNA was prepared using the RNeasy Micro kit (Qiagen). cDNA was prepared and amplified from 2 ng of total RNA using the Ovation RNA-Seq System V2 (NuGEN). Amplified cDNA was fragmented to an average of 200–300 bp before ligating to barcoded-TruSeq adaptors using the Encore Rapid Library System (NuGEN). Libraries were pooled and sequenced for >5 × 107 reads on a HiSeq 2000 (Illumina). Fastq files were obtained after demultiplexing with CASAVA (v1.8.2) and aligned to the reference mouse genome (mm9) using tophat v1.3 (Trapnell et al., 2009). Differential expression was determined with U-Seq version 8.0.2 (Nix et al., 2008).

Bioinformatics

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Previously published ChIP-seq datasets available as BigWig files (Telese et al., 2015) were uploaded and visualized on the UCSC Genome Browser. For comparative sequence analyses of evolutionary conservation in the Plxna4 locus and identification of conserved MEF2 sites, the Evolutionary Conserved Regions (ECR) Browser suite of tools was used (https://rvista.dcode.org) (Frazer et al., 2004).

Collagen gel explant culture

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E14.5 STG were dissected in PBS, cut into several pieces and placed into a rat-tail-collagen gel as described previously (Manousiouthakis et al., 2014). For STG-dorsal aorta co-culture, E14.5 STG and thoracic aorta segments were separately dissected from Ednra-/-, Th-Cre/Ednrafl/- and their littermate controls. Control, Ednra-/-, Th-Cre/Ednrafl/- STG were placed in a collagen gel at the proximity of the thoracic aorta segments of the indicated genotype and grown in L15-CO2 medium supplemented with 10% FBS for 3 days, then fixed with 4% PFA. Neurite outgrowth was evaluated by immunostaining the explants with anti-Th (1:400; Millipore AB1542) antibody followed by detection using Alexa Fluor secondary antibodies (Life Science). To quantify neurite outgrowth, the fluorescent labeled neurites extending from explants were measured by binary threshold selection using Fiji-Image J software.

For STG-COS aggregate co-culture, COS7 (ATCC CRL-1651, LOT: 5784927) cell aggregates were prepared in 40 μl hanging drops of 5 × 105 cells/ml suspension of untransfected or Ad-GFP-2A-mSema3A (VectorBio ADV-271580) transfected COS cells for 3 days at 37°C. Separately, E14.5 STGs were dissected from Ednra-/-, Plxna4-/- and their littermate controls. Control, Ednra-/-, Plxna4-/- STGs were placed in a collagen gel at the proximity of untransfected-COS cell aggregates or between untransfected- and Sema3a-transfected-COS cell aggregates, and grown in L15-CO2 medium supplemented with 10% FBS for 4 days. Neurite outgrowth was evaluated as described above.

Quantitative real-time RT-PCR

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Single STGs were dissected individually from E14.5 Ednra, Edn1 and Ece1 mutants and their littermate control embryos. Total RNA was extracted from individual STG by guanidinium isothiocyanate extraction and reverse transcribed using M-MLV reverse transcriptase. All samples were analyzed independently by real-time PCR using iCycler iQ with SYBR green supermix (Bio-Rad) with the following primer pairs; hprt (primer bank ID: 7305155a1, 5’-TCAGTCAACGGGGGACATAAA-3’, 5’-GGGGCTGTACTGCTTAACCAG-3’), nrp1 (primer bank ID: 6679134a1, 5’-GACAAATGTGGCGGGACCATA-3’, 5’-TGGATTAGCCATTCACACTTCTC-3’), plxna3 (primer bank ID: 667939a1, 5’-CAGATACCACTCTGACTCACCT-3’, 5’-GGCCCGTAGCTCAGTTAGG-3’), plxna4 (primer bank ID: 28461143a1, 5’-ACAGGGCACATTTATTTGGGG-3’, 5’-CACTTGGGGTTGTCCTCATCT-3’).

Electrocardiography (ECG)

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6–7 week-old mice were anesthetized by isoflurane inhalation via a SomnoSuite small animal anesthesia system (Kent Scientific), and needle electrodes were inserted subcutaneously in a standard lead II arrangement (at the right thoracic limb and the left pelvic limb) to obtain ECG readings with a Powerlab 35 data acquisition system (AD Instruments). Once stable baseline heart rate was confirmed, drug was administered by intraperitoneal injection. Dosage of drug used was 2 mg/kg for amphetamine, 10 μg/kg for isoproterenol, and 25 μg/kg for propranolol. The ECG for each subject was recorded continuously for the entire period of the experiment. LabChart eight software (AD Instruments) was used for heart rate and heart rate variability analyses.

Statistics

All quantified data were graphed as mean ± s.e.m. or mean ± s.d., and analyzed for significance using an unpaired Student’s t-test. Minimum sample sizes were determined based on population size, confidence level and standard errors/deviations.

Data availability

Previously published ChIP-seq datasets available as BigWig files (Telese et al. 2015) were uploaded and visualized on the UCSC Genome Browser.

The following previously published data sets were used
    1. Telese F
    2. Ma Q
    3. Perez PM
    4. Notani D
    5. Oh S
    6. Li W
    7. Comoletti D
    (2015) NCBI Gene Expression Omnibus
    ID GSE66710. LRP8-Reelin-Regulated Neuronal Enhancer Signature Underlying Learning and Memory Formation.
    https://www.ncbi.nlm.nih.gov/geo/query/acc.cgi?acc=GSE66710

References

    1. Clouthier DE
    2. Hosoda K
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Article and author information

Author details

  1. Denise M Poltavski

    The Saban Research Institute, Children’s Hospital Los Angeles, University of Southern California Keck School of Medicine, Los Angeles, United States
    Contribution
    Data curation, Formal analysis, Validation, Investigation, Visualization, Methodology, Writing—original draft, Writing—review and editing
    Competing interests
    No competing interests declared

  2. Pauline Colombier

    Cardiovascular Research Institute, University of California, San Francisco, San Francisco, United States
    Contribution
    Resources, Data curation, Software, Formal analysis, Validation, Investigation, Methodology, Writing—review and editing
    Competing interests
    No competing interests declared

  3. Jianxin Hu

    Cardiovascular Research Institute, University of California, San Francisco, San Francisco, United States
    Contribution
    Data curation, Formal analysis
    Competing interests
    No competing interests declared

  4. Alicia Duron

    1. The Saban Research Institute, Children’s Hospital Los Angeles, University of Southern California Keck School of Medicine, Los Angeles, United States
    2. Darby Children’s Research Institute, Department of Pediatrics, Medical University of South Carolina, Charleston, United States
    Contribution
    Data curation, Validation
    Competing interests
    No competing interests declared

  5. Brian L Black

    Cardiovascular Research Institute, University of California, San Francisco, San Francisco, United States
    Contribution
    Resources, Data curation, Software, Formal analysis, Supervision, Funding acquisition, Validation, Investigation, Visualization, Methodology, Writing—review and editing
    Competing interests
    No competing interests declared
    ORCID icon "This ORCID iD identifies the author of this article:" 0000-0002-6664-8913

  6. Takako Makita

    1. The Saban Research Institute, Children’s Hospital Los Angeles, University of Southern California Keck School of Medicine, Los Angeles, United States
    2. Darby Children’s Research Institute, Department of Pediatrics, Medical University of South Carolina, Charleston, United States
    Contribution
    Conceptualization, Resources, Data curation, Software, Formal analysis, Supervision, Funding acquisition, Validation, Investigation, Visualization, Methodology, Writing—original draft, Project administration, Writing—review and editing
    For correspondence
    makita@musc.edu
    Competing interests
    No competing interests declared
    ORCID icon "This ORCID iD identifies the author of this article:" 0000-0002-5598-5690

Funding

National Institute of Neurological Disorders and Stroke (NS062901)

  • Takako Makita

National Institute of Neurological Disorders and Stroke (NS083265)

  • Takako Makita

National Heart, Lung, and Blood Institute (HL064658)

  • Brian L Black

National Heart, Lung, and Blood Institute (HL136182)

  • Brian L Black

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

Acknowledgements

We thank Catherine Bridges and Chris Cowan for provision of additional Mef2c mutant embryos to complete this study. This research was supported by grants NS062901 and NS083265 from National Institutes of Health to TM, and by grants HL064658 and HL136182 from National Institutes of Health to BLB.

Ethics

Animal experimentation: All experiments with animals complied with National Institute of Health guidelines and were reviewed and approved by the Children's Hospital Los Angeles (274-18), UCSF (AN171342) or MUSC (2018-00627) Institutional Animal Care and Use Committee.

Copyright

© 2019, Poltavski 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.

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  1. Denise M Poltavski
  2. Pauline Colombier
  3. Jianxin Hu
  4. Alicia Duron
  5. Brian L Black
  6. Takako Makita
(2019)
Venous endothelin modulates responsiveness of cardiac sympathetic axons to arterial semaphorin
eLife 8:e42528.
https://doi.org/10.7554/eLife.42528

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https://doi.org/10.7554/eLife.42528

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