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Logo of jcinvestThe Journal of Clinical InvestigationCurrent IssueArchiveSubscriptionAbout the Journal
J Clin Invest. 2011 May 2; 121(5): 1974–1985.
Published online 2011 April 18. doi:  10.1172/JCI44900
PMCID: PMC3083763

Sema3E-PlexinD1 signaling selectively suppresses disoriented angiogenesis in ischemic retinopathy in mice


During development, the retinal vasculature grows toward hypoxic areas in an organized fashion. By contrast, in ischemic retinopathies, new blood vessels grow out of the retinal surfaces without ameliorating retinal hypoxia. Restoration of proper angiogenic directionality would be of great benefit to reoxygenize the ischemic retina and resolve disease pathogenesis. Here, we show that binding of the semaphorin 3E (Sema3E) ligand to the transmembrane PlexinD1 receptor initiates a signaling pathway that normalizes angiogenic directionality in both developing retinas and ischemic retinopathy. In developing mouse retinas, inhibition of VEGF signaling resulted in downregulation of endothelial PlexinD1 expression, suggesting that astrocyte-derived VEGF normally promotes PlexinD1 expression in growing blood vessels. Neuron-derived Sema3E signaled to PlexinD1 and activated the small GTPase RhoJ in ECs, thereby counteracting VEGF-induced filopodia projections and defining the retinal vascular pathfinding. In a mouse model of ischemic retinopathy, enhanced expression of PlexinD1 and RhoJ in extraretinal vessels prevented VEGF-induced disoriented projections of the endothelial filopodia. Remarkably, intravitreal administration of Sema3E protein selectively suppressed extraretinal vascular outgrowth without affecting the desired regeneration of the retinal vasculature. Our study suggests a new paradigm for vascular regeneration therapy that guides angiogenesis precisely toward the ischemic retina.


In ischemic retinopathies, including proliferative diabetic retinopathy (PDR) and retinopathy of prematurity (ROP), hypoxia that follows retinal capillary obliteration drives deregulated growth of new blood vessels protruding out of the retinal surfaces, without ameliorating retinal ischemia (13). Sustained hypoxia further exacerbates extraretinal vascular outgrowth, which can cause vision-impairing hemorrhage and retinal detachment. Therefore, it has been widely assumed that blood vessel formation per se should be prevented to treat these common blinding diseases (4). A series of anti-VEGF drugs are now being clinically evaluated for their antiangiogenic potency in treating PDR and ROP (5, 6). However, to fundamentally resolve disease pathogenesis, the promotion of properly guided angiogenesis to reoxygenize the ischemic retina would be of far greater benefit. In this context, it is crucial to identify the molecular targets that can selectively prevent disoriented angiogenesis and thus facilitate retinal vascular regeneration.

For the elaboration of therapies to guide new blood vessels toward the hypoxic retina, the molecular mechanisms underlying intraretinal angiogenesis during developmental periods provide invaluable information. In developing mouse retinas, astrocytes trigger postnatal onset of radial vascular extension from the optic disc by secreting VEGF (also known as VEGF-A) and depositing ECM scaffolds to which the migrating ECs adhere (7, 8). Subsequently, a monolayered vascular network is formed over the superficial retinal area within the first postnatal week. In this process, the concentration gradients of VEGF proteins along the preexisting astrocyte network promote the projection of endothelial filopodia from the tips of sprouting vessels, thereby determining angiogenic orientation (9). On the other hand, diffusible VEGF proteins may induce disoriented filopodia projections (9, 10), which should be pruned to restrict retinal vascular pathfinding.

To date, several signaling molecules that guide axonal pathfinding have also been shown to participate in the control of angiogenic orientation (11). In particular, direct binding of the soluble semaphorin 3E (Sema3E) ligand to the transmembrane PlexinD1 receptor, which can act as either an attractive or repulsive cue on neurite extension (12, 13), mediates filopodium retraction in growing blood vessels (14) by inactivating R-Ras and activating Arf6 small GTPases (15, 16), which leads to the disassembly of integrin-mediated adhesive structures. However, the question remains: how does Sema3E-PlexinD1 signaling cooperate with VEGF signaling in defining vascular pathfinding in developing retinas? Moreover, little is known about what signaling defects are responsible for the disoriented vascular outgrowth in ischemic retinopathies.

Here we show that ECs of the developing retinal vessels express PlexinD1 in response to VEGF signaling. Neuron-derived Sema3E signals via PlexinD1 and counteracts VEGF-induced projection of endothelial filopodia by activating the small GTPase RhoJ. In a mouse model of ischemic retinopathy, prominent expression of endothelial PlexinD1 and RhoJ was limited to the abnormal extraretinal vessels. By targeting PlexinD1, intravitreal injection of Sema3E protein selectively suppressed disoriented outgrowth of extraretinal vessels, leading to the subsequent regeneration of normal vasculature in ischemic retinas.


ECs express PlexinD1 in response to VEGF signaling in the developing retinal vasculature.

To explore a therapeutic approach that restores proper angiogenic orientation in ischemic retinopathies, we attempted to exploit the molecular mechanisms underlying intraretinal angiogenesis during development, with special attention to those regulating endothelial filopodia projections. Starting from this framework, we initiated our study by detecting the spatial association of PlexinD1-expressing ECs with VEGF-expressing astrocytes in P4 mouse retinas, in which blood vessels were growing within the superficial area. As previously reported (9, 10, 17), the Vegf gene was strongly expressed in retinal astrocytes ahead of the advancing vascular fronts, while moderate Vegf expression was maintained around the preformed capillaries and veins, but not around arteries (Figure (Figure1,1, A and B). This expression pattern of the Vegf gene can be ascribed to different oxygen concentrations depending on the type of vessel (18). By contrast, the Plxnd1 gene is strongly expressed in ECs located at the tips and in the stalks of sprouting vessels (Figure (Figure1,1, C and D). In addition, Plxnd1 is moderately expressed in preformed capillaries and veins, but not in arteries (Figure (Figure1C).1C). Thus, it seems likely that PlexinD1-expressing ECs reside adjacent to VEGF-expressing astrocytes. To determine whether the expression level of the endothelial Plxnd1 gene fluctuates by manipulating VEGF signaling, we examined Plxnd1 expression after intravitreal injection of a soluble VEGFR1 protein (VEGFR1-Fc), which functions as a high-affinity decoy receptor for VEGF (19). After VEGFR1-Fc injection, endothelial Plxnd1 expression was downregulated at around 7 hours (Supplemental Figure 1; supplemental material available online with this article; doi: 10.1172/JCI44900DS1), and became undetectable at 8 hours throughout the developing retinal vasculature (Figure (Figure1E).1E). These results indicate that ECs express PlexinD1 in response to VEGF signaling in growing retinal vessels.

Figure 1
ECs express PlexinD1 in response to VEGF signaling in the developing retinal vasculature.

PlexinD1 signaling counteracts VEGF-induced projections of endothelial filopodia.

To determine the role of PlexinD1 signaling in retinal vascular development, we pharmacologically neutralized its endogenous ligands by intravitreal injection of its soluble protein, PlexinD1-Fc (20). Five hours after PlexinD1-Fc injection at P5, we observed an increase in the length and number of endothelial filopodia, both at the tips and in the stalks of the sprouting vessels (Figure (Figure2,2, A and B). Furthermore, consistent with the endothelial PlexinD1 distribution, numerous filopodia ectopically projected from the preformed capillaries around veins, but not arteries (Figure (Figure2A).2A). Thus, ECs, be they at the tips or in the stalks of sprouting retinal vessels, can elongate filopodia, and this is constitutively suppressed by PlexinD1 signaling. To further examine the contribution of PlexinD1 signaling to retinal vascular patterning, we examined the P5 retinal vasculature 48 hours after intravitreal PlexinD1-Fc injection at P3. This treatment led to the formation of a multilayered capillary network crossing over and under the veins (Figure (Figure2A).2A). By contrast, neutralization of endogenous VEGF rapidly depleted the endothelial filopodia throughout the developing retinal vasculature, which subsequently led to the abrogation of the capillary network (Figure (Figure2,2, A and B). These results illustrate that the fine-tuning of endothelial filopodia regulated by VEGF and PlexinD1 signaling is a prerequisite for organizing the retinal vascular architecture.

Figure 2
PlexinD1 signaling retracts endothelial filopodia in retinal vascular development.

Neuron-derived Sema3E restricts vascular pathfinding in developing retinas.

Based on a previous study demonstrating identical vascular defects in mouse embryos deficient for the Plxnd1 and Sema3e genes (14), we next assessed the role of Sema3E in retinal vascular development. At P4, while the Plxnd1 gene was expressed in vascular ECs and in a small subset (7.4%) of underlying neurons in the ganglion cell layer (GCL), the Sema3e gene was expressed in 37% of neurons throughout the GCL (Figure (Figure3A).3A). Intravitreal injection of the Sema3E–alkaline phosphatase (Sema3E-AP) fusion protein, which can bind directly to PlexinD1 (14), identified its targets on the ECs of growing retinal vessels (Figure (Figure3B).3B). Because PlexinD1 is a primary receptor for Sema3E (14), these findings indicate that neuron-derived Sema3E acts on the overlying ECs expressing PlexinD1. In P4 retinas of Sema3e-deficient (Sema3e–/–) mice, the retinal vascular patterning displayed a wide variety of morphological defects, including solitary clusters of retinal ECs isolated from the advancing vascular fronts, attachment of hyaloid vessels to the retinal surface, and disorganized remodeling into distinct arteries, veins, and capillaries (Figure (Figure3C3C and Supplemental Figure 2). While the length of endothelial filopodia was significantly increased in Sema3e–/– mice compared with that in Sema3e+/– mice, the overall vascular density was significantly decreased in Sema3e–/– retinas (Figure (Figure3D),3D), which seems inconsistent with that seen in P5 retinas injected with the PlexinD1-Fc protein at P3 (Figure (Figure2,2, A and B). Nonetheless, the vascular phenotypes in Sema3e–/– retinas were reproduced by PlexinD1-Fc injection at P1 (Supplemental Figure 2I), which neutralized endogenous ligands for PlexinD1 throughout the entire process of retinal vascular development. Of note, we observed ectopic vascular invasion into the GCL of Sema3e–/– mice (Figure (Figure3E),3E), suggesting that diffusion of Sema3E prevents misdirected vertical projections of endothelial filopodia, thereby facilitating the horizontal extension of the monolayered vascular network in the superficial retinal area (Figure (Figure3F). 3F).

Figure 3
Neuron-derived Sema3E restricts vascular pathfinding in developing retinas.

Sema3E-induced activation of the small GTPase RhoJ retracts endothelial filopodia.

To determine the molecular mechanisms underlying the counteracting property of Sema3E-PlexinD1 signaling in terms of VEGF-induced filopodia projections, we sought out endothelial Rho small GTPases, intracellular molecular switches for the cytoskeletal rearrangements that comprise more than 20 different proteins (2123). By performing microarray gene expression analyses exploiting ECs sorted from neonatal mouse retinas in conjunction with whole-mount retinal in situ hybridization (ISH), we found that the Rhoj gene (also known as Tc10-like [Tcl], ref. 24, and previously referred to as Rhot; ref. 25) was expressed almost exclusively in ECs in developing retinas (Figure (Figure4A).4A). Interestingly, endothelial Rhoj expression was prominent in veins and capillaries of growing retinal vessels, but was downregulated at later postnatal stages, which synchronized with the Plxnd1 expression (Supplemental Figure 3). Based on its protein structure, RhoJ is categorized into the Cdc42 small GTPase subfamily (26, 27), and it was previously reported that RhoJ induces filopodia projections in cultured neuronal cells (25). However, in cultured HUVECs, ectopic expression of the wild-type RhoJ (RhoJ-WT) and its constitutively active form (RhoJ-CA), but not the dominant-negative form (RhoJ-DN), induced cell contraction with reduction of stress fibers (Figure (Figure4,4, B and D, and Supplemental Figure 4A; see also Supplemental Video 1). Of note, ectopically expressed RhoJ-WT proteins accumulated in the membrane blebs, to which endogenous RhoJ proteins were also localized after Sema3E stimulation (Supplemental Figure 4B). This contrasts with the cytoplasmic localization of RhoJ proteins in normal or VEGF-stimulated HUVECs (Supplemental Figure 4B). Intriguingly, Sema3E-induced cell contraction was abolished by knockdown of RhoJ with siRNA (Figure (Figure4,4, C and D, and Supplemental Figure 4C; see also Supplemental Videos 2–4), indicating that RhoJ is a pivotal intracellular molecule that mediates Sema3E-induced retraction of endothelial filopodia. Indeed, RhoJ was inactivated by VEGF, but activation was restored by exposure to Sema3E (Figure (Figure4E).4E). Thus, RhoJ is the common downstream target of the VEGF and Sema3E signals in regulating endothelial cytoskeletal rearrangements (Figure (Figure4F). 4F).

Figure 4
Sema3E-induced activation of the small GTPase RhoJ retracts endothelial filopodia.

To further evaluate the role of RhoJ in retinal vascular development, we used a gain-of-function gene-targeting approach. For this purpose, we inserted a cDNA encoding the murine wild-type Rhoj gene, preceded by the synthetic CAG promoter (28) and a loxP-flanked Neor-STOP cassette, into the ubiquitously expressed Rosa26 locus (ref. 29 and Supplemental Figure 5A). We crossed these conditional Tg mice carrying the allele termed R26-Rhoj to Tie2Cre Tg mice (30) to obtain offspring overexpressing RhoJ in ECs. After mating Tie2CreTg/WTR26-RhojTg/WT male with R26-RhojTg/Tg female mice, we could not obtain Tie2CreTg/WTR26-RhojTg/Tg neonates (Supplemental Figure 5B), indicating their embryonic lethality because of endothelial RhoJ overexpression. Indeed, Tie2CreTg/WTR26-RhojTg/Tg embryos at 10.5 dpc demonstrated growth retardation, with defective vascular development (Supplemental Figure 5C). We therefore attempted to analyze retinal vascular development in Tie2CreTg/WTR26-RhojTg/WT neonates, in which endothelial RhoJ overexpression was monitored by the bicistronic expression of EGFP upon excision of the Neor-STOP cassette (Figure (Figure4G4G and Supplemental Figure 5D). Consistent with the ectopic RhoJ expression in cultured HUVECs, we observed numerous membrane blebs formed in ECs of sprouting retinal vessels (Figure (Figure4H).4H). This was also observed in inducible RhoJ overexpression in ECs after systemic administration of 4-hydroxytamoxifen (4OHT) to CAG-MerCreMer mice (31) carrying the R26-Rhoj allele (Figure (Figure4I).4I). Because endothelial filopodia projections were not apparently affected in RhoJ-overexpressing ECs, the membrane blebbing implied the fast cycling of projection and retraction of endothelial filopodia.

Extraretinal vessels highly express PlexinD1 and RhoJ in ischemic retinas.

With the molecular machinery underlying the intraretinal angiogenesis in mind, we next attempted to unveil the etiological process of extraretinal angiogenesis in ischemic retinopathies. For this purpose, we examined the spatial distribution of cells expressing Vegf, Sema3e, Plxnd1, and Rhoj genes in a mouse model of oxygen-induced retinopathy (OIR) (32). In this model, the mouse pups were housed in a hyperoxic state from P7 to P12, resulting in the regression of preformed capillaries in the central retinal areas (Supplemental Figure 6A). When the pups were returned to normal room air, the arising hypoxia induced vascular regrowth from the remaining vessels toward the ischemic retinas. At around P15, while retinal revascularization proceeded, new blood vessels protruded out of the retinal surfaces, as seen in human ischemic retinopathies. At P16, Vegf expression was almost absent in astrocytes, unlike during development (Figure (Figure5,5, A–C). Instead, a considerable number of the underlying neurons in ischemic retinal areas expressed Vegf. By contrast, Sema3e was broadly scattered across neurons throughout the GCL (Figure (Figure5,5, D–F), as seen in normal retinas (Supplemental Figure 3). Intriguingly, the ECs of extraretinal vessels highly expressed the Plxnd1 gene, while its expression was hardly detectable in intraretinal vessels (Figure (Figure5,5, G–I). Likewise, prominent Rhoj expression was limited to the extraretinal vessels (Figure (Figure5,5, J–L). These findings suggest that neuron-derived Sema3E signals to endothelial PlexinD1 and activates RhoJ restrictively in extraretinal vessels.

Figure 5
Extraretinal vessels highly express PlexinD1 and RhoJ in ischemic retinas.

PlexinD1 signaling suppresses extraretinal vascular outgrowth in ischemic retinas.

Because neuron-derived Sema3E prevents downward vascular growth in developing retinas, we suspected that diffusion of Sema3E through the superficial retinal areas might force the PlexinD1-expressing ECs out of the retinal surfaces in the OIR model (Figure (Figure6A).6A). Unexpectedly, however, 24 hours after intravitreal injection of PlexinD1-Fc at P14, we observed extraretinal projections of numerous filopodia (Figure (Figure6B).6B). By contrast, VEGFR1-Fc injection completely abolished extraretinal vascular outgrowth, while discrete fragments of intraretinal ECs implied progressive vascular regression (Figure (Figure6B). 6B).

Figure 6
PlexinD1 signaling counteracts VEGF-induced extraretinal vascular outgrowth in ischemic retinas.

To further assess the roles of VEGF and PlexinD1 signaling in the construction of the disorganized vascular architecture in the OIR model, we inactivated the genes Vegfr2 and Plxnd1, encoding endothelial receptors, using tamoxifen-inducible Cre-loxP–mediated genetic recombination (Supplemental Figure 6, B and C). After daily systemic administration of 4OHT to CAG-MerCreMer mice carrying loxP-flanked (33) and constitutive null (34) alleles for the Vegfr2 (Vegfr2flox/–) gene, we observed complete depletion of the extraretinal vessels (Figure (Figure6,6, C and D). Concurrently, the intraretinal vascular regeneration was also interrupted, leading to a substantial decrease in capillary density, with large unvascularized retinal areas (Supplemental Figure 7). By contrast, inducible inactivation of the Plxnd1 gene (14, 35) led to a conspicuous increase in the number of extraretinal vessels, while intraretinal vascular regeneration proceeded as in the control retina (Figure (Figure6,6, C and D). Consistent with the notion that RhoJ acts as a downstream molecule of PlexinD1 signaling, inducible RhoJ overexpression in the OIR mice resulted in a significant decrease in the number of extraretinal vessels, while intraretinal capillary density was also reduced (Figure (Figure6,6, C and D). These results together indicate that PlexinD1 signaling protects blood vessels in ischemic retinas from VEGF-induced extraretinal vascular outgrowth.

Intravitreal Sema3E protein restores proper angiogenic orientation in ischemic retinas.

Based on the findings described above, we hypothesized that diffusion of neuron-derived Sema3E into the preretinal space might act on extraretinal PlexinD1 but is insufficient to fully suppress VEGF-induced disoriented angiogenesis in ischemic retinopathy. Therefore, to directly stimulate PlexinD1 in the extraretinal vessels, we injected Sema3E protein into the vitreous space at P14 in the OIR model. At 24 hours after injecting 1 μl of Sema3E protein at a concentration of 2 μg/μl, we found no apparent effects on intraretinal filopodia projections (Figure (Figure7A),7A), which was attributed to the lack of PlexinD1 expression in these ECs. However, at 72 hours after this treatment, we observed a significant decrease in extraretinal vessels (Figure (Figure7,7, B and C). Notably, this effect was more pronounced, without reducing intraretinal capillary density, after injection of Sema3E protein at a higher concentration (Figure (Figure7C7C and Supplemental Figure 8). The newly formed intraretinal vessels were almost uniformly associated with periendothelial mural cells (Supplemental Figure 9). Thus, the intravitreal Sema3E injection led to the regeneration of the normal vascular architecture by restoring angiogenic orientation in ischemic retinas. By contrast, VEGFR1-Fc injection suppressed the intraretinal projections of endothelial filopodia (Figure (Figure7A),7A), with concomitant regression of the remaining capillaries (Supplemental Figure 9), which resulted in extensive ischemic retinal areas (Figure (Figure7,7, B and C, and Supplemental Figure 8).

Figure 7
Intravitreal Sema3E injection selectively suppresses extraretinal vascular outgrowth without affecting vascular regeneration in ischemic retinas.


Anti-VEGF drugs have been reported to temporarily halt disease progression in some refractory cases of ischemic retinopathies (5, 6). This pharmacological approach has offered a breakthrough that obviates destructive therapies such as laser photocoagulation and surgical interventions. However, as shown in our study, comprehensive inhibition of angiogenesis may sustain retinal ischemia, which will consequently exacerbate disordered angiogenesis unless the anti-VEGF drugs are repeatedly administered. To overcome this limitation, we postulated that normalization of angiogenic orientation will offer an alternative, but effective treatment to fundamentally resolve retinal ischemia. Starting from this premise, we explored a therapeutic approach that can selectively suppress disoriented angiogenesis by exploiting the molecular mechanisms underlying intraretinal angiogenesis during development.

In postnatal mouse retinas, we observed an intimate association between PlexinD1-expressing ECs and VEGF-expressing astrocytes, which was corroborated by Plxnd1 gene downregulation after blocking VEGF signaling. While blocking PlexinD1 signaling rapidly elongated endothelial filopodia, the disruption of Sema3e, which is expressed in neurons in the GCL, caused defective patterning of the retinal vasculature. Based on these findings, we propose that Sema3E-PlexinD1 signaling acts as a negative feedback system against VEGF signaling in terms of the filopodia projections as follows: Under hypoxia, VEGF evokes a series of proangiogenic signaling cascades for proliferation, survival, and migration (36) but simultaneously upregulates PlexinD1 expression. Sema3E diffusing from the underlying neurons constantly signals to endothelial PlexinD1. ECs can project filopodia when VEGF signaling rises above the threshold level defined by the PlexinD1 signaling.

In the present study, we showed for the first time to our knowledge that Sema3E-induced activation of RhoJ mediates endothelial contraction. This contrasts with VEGF-induced activation of Cdc42 (37), which plays a crucial role in filopodia projections (26, 27). Interestingly, RhoJ and Cdc42 were inactivated by VEGF and Sema3E, respectively (Supplemental Figure 10A). Thus, it seems likely that VEGF and Sema3E signals inversely activate or inactivate Cdc42 and RhoJ. Upon activation, both RhoJ and Cdc42 bind to the Cdc42/Rac-interactive binding (CRIB) domains of their effector proteins, such as p21-activated kinase (PAK) and neural Wiskott-Aldrich syndrome protein (N-WASP), which regulate intracellular actin polymerization (24, 25). Given the opposite effects of RhoJ and Cdc42 on endothelial filopodia formation, we suggest that activated RhoJ and Cdc42 competitively bind to their effector proteins, whereby the endothelial filopodia project or retract (Supplemental Figure 10B). Considering the expression of Cdc42 in various types of cells, the endothelial expression of RhoJ indicates the possibility that this molecule could serve as a therapeutic target to specifically manipulate endothelial filopodia projections.

Given the molecular machinery described above, one may ask how such a fine-tuning of endothelial filopodia projections contributes to the establishment of the retinal vascular architecture. A key to answering this question may be the contradictory consequences of filopodia elongation after PlexinD1-Fc injections at different time points. PlexinD1-Fc injection at P3 led to the formation of an excessive capillary network around veins, whereas its injection at P1 resulted in a sparse capillary network with less apparent morphological distinction between arteries and veins. This discrepancy may partly be explained by the extent of preformed vessels at the time of PlexinD1-Fc injection. That is, elongated filopodia may fuse extensively with neighboring vessels after P3, when the retinal vascular network has been considerably formed. By contrast, when PlexinD1 signaling is blocked just after the onset of the retinal vascular development, the aberrantly projected filopodia may fail to anastomose with each other, leading to the formation of a discontinuous capillary network. In line with this idea, the overall vascular density was decreased in Sema3e-deficient retinas, despite the increased length of endothelial filopodia. Of importance, the Sema3e-deficient retinas demonstrated a wide variety of vascular defects in their extent as well as in their morphological phenotypes, which is ascribable to the functional redundancy of endogenous ligands for PlexinD1. While Sema3E is the only ligand that can directly bind to PlexinD1, other soluble Sema3 ligands may signal to PlexinD1 in the co-presence of neuropilins (38), to compensate for the loss of Sema3E or to exert their distinct functions.

In postnatal mouse retinas, developing vessels grow without protruding out of the retinal surface, even after pharmacological blockade of PlexinD1 or genetic disruption of Sema3e. This excludes the possibility that a deficiency in Sema3E-PlexinD1 signaling alone is sufficient for extraretinal angiogenesis. By contrast, overexpression of soluble VEGF can cause extraretinal projections of endothelial filopodia in developing retinal vasculature (9). As we showed the complete suppression of extraretinal angiogenesis by pharmacological or genetic disruption of VEGF signaling in the OIR model, it seems likely that aberrant VEGF distribution is primarily responsible for extraretinal angiogenesis. Indeed, the predominant VEGF-expressing cells in the OIR model are neurons rather than astrocytes. In addition, astrocytes failed to deposit extracellular fibronectin matrices (Supplemental Figure 11), which may have led to the loss of physical scaffolds for migrating ECs and the inability to retain heparin-binding VEGF proteins within the retina. The resulting diffusion and accumulation of VEGF in the preretinal space, as documented in human ischemic retinopathies (39), may induce disoriented extraretinal vascular outgrowth. In this context, a high VEGF concentration accounts for the elevated PlexinD1 expression in extraretinal vessels.

By exploiting the differential distribution of PlexinD1 in the OIR model, we showed that intravitreal Sema3E injection selectively prevented extraretinal vascular outgrowth. Because of the absence of PlexinD1 expression in intraretinal vessels, this treatment did not interfere with vascular regeneration in ischemic retinas. To date, experimental manipulation of various signaling molecules, such as inducible nitric oxide synthase (40) and sphingosine 1–phosphatase (41), has been demonstrated to successfully prevent or repair vascular abnormalities in OIR models. Nonetheless, it is intriguing that diffuse administration of soluble Sema3E proteins can correct the imbalance in the complex signaling machineries determining retinal angiogenic orientation. This simplicity may allow clinical adaptation of this treatment for vascular regeneration therapy in ischemic retinopathies.

The feasibility of intravitreal Sema3E therapy is further supported by the specific involvement of PlexinD1 signaling in angiogenic sprouting, which will lessen the undesirable effects on normal vascular functions. However, the expression of PlexinD1 in neurons, although only limited to a small population in the GCL, suggests that caution must be exercised regarding the direct effects of Sema3E on retinal neurons, especially in clinical use for premature infants, whose retinal neural networks may not have been fully established (42). Indeed, in Sema3e–/– mice, we occasionally observed disordered axonal fibers in small retinal areas (Supplemental Figure 12), implying a role for Sema3E in axonal pathfinding in specific populations of retinal ganglion cells. While we demonstrated dose-dependent efficacy of intravitreal Sema3E injection in suppressing disoriented angiogenesis, its appropriate dosage remains to be determined to minimize the potential undesirable effects.

Further studies are needed to evaluate whether intravitreal Sema3E administration alone can offer vascular regeneration therapy in ischemic retinopathies, because this treatment did not reduce the unvascularized retinal areas in the OIR model. In some cases of human ROP, in which physiological retinal angiogenesis spontaneously recurs, it has been clinically reported that intravitreal anti-VEGF therapy paradoxically promotes physiological angiogenesis (6). Nevertheless, our experimental results demonstrated that VEGFR1-Fc injection, irrespective of Sema3E coinjection, comprehensively inhibited vascular regrowth in the OIR model (Supplemental Figure 8), indicating the clinical requirements for restricted use of anti-VEGF drugs in severe ROP. Also, in human PDR, which often lacks spontaneous vascular regeneration in ischemic retinas, selective suppression of extraretinal angiogenesis by Sema3E injection will be more beneficial when conjugated with additional modalities that promote intraretinal vascular growth, such as restoration of proangiogenic properties in retinal astrocytes (43).

In conclusion, we have presented a paradigm of vascular regeneration therapy in ischemic retinas by exploiting the antiangiogenic action of Sema3E on PlexinD1-expressing extraretinal vessels. Sema3E administration can also be useful to precisely guide angiogenesis to ischemic tissues in other organs if PlexinD1 expression is restricted to disoriented vessels. Otherwise, in diseases with broad PlexinD1 expression in abnormal vessels, such as cancer (44), Sema3E administration may be a potent antiangiogenic therapy. Thus, the outcomes of Sema3E therapy may depend on the distribution of endothelial PlexinD1 in distinct disease settings.



Analyses of retinal vascular development were performed in WT mice with ICR or C57BL/6 backgrounds (SLC Japan). For the generation of R26-Rhoj Tg mice (RIKEN CDB acc. no. CDB0919K;, a cDNA encoding a native form of murine Rhoj was cloned into a modified version of pROSA26-1 vector (29) (provided by Y. Sasaki, RIKEN CDB), preceded by the ubiquitous CAG promoter (28) and a loxP-flanked Neor-STOP cassette, followed by a frt-flanked IRES-EGFP cassette and a bovine polyadenylation sequence (Supplemental Figure 5A). Gene targeting was done with TT2 ES cells and confirmed by Southern blotting. Mice were generated by injection of targeted ES cells into ICR embryos and backcrossed with the C57BL/6 strain. PCR genotyping was performed with forward primer R26F2 (5′-AAAGTCGCTCTGAGTTGTTAT-3′) and reverse primer R1295 (5′-GCGAAGAGTTTGTCCTCAACC-3′) (product size of 303 bp for the R26-Rhoj allele) and reverse primer R523 (5′-GGAGCGGGAGAAATGGATATG-3′) (product size of 601 bp for the WT allele). Female mice carrying the R26-Rhoj allele were bred with Tie2Cre (30) male mice (provided by R. Wang, UCSF, San Francisco, California, USA), to delete the Neor-STOP cassette and drive RhoJ expression in ECs. Frozen embryos of Sema3e-deficient mice (14) with a C57BL/6 background (European Mouse Mutant Archive ID, EM:01373) were provided by C.E. Henderson, Columbia University, New York, New York, USA. CAG-MerCreMer Tg mice (31) (RIKEN CDB acc. no. CDB0404T) were mated with Plxnd1-deficient (14) and Plxnd1-floxed (35) (provided by T.M. Jessell, Columbia University, New York, New York, USA), Vegfr2-deficient (34) and Vegfr2-floxed (33) (provided by J. Rossant, Hospital for Sick Children Research Institute, Toronto, Canada), and R26-Rhoj mice with C57BL/6 backgrounds to obtain tamoxifen-inducible conditional mutants. Cre-loxP–mediated genetic recombination in the OIR model was induced by i.p. injections of 30 μl of 10 mg/ml 4OHT (Sigma-Aldrich) dissolved in 1:9 ethanol/sunflower oil (Sigma-Aldrich) once daily from P12 after return to normal room air. The OIR model was established by maintaining the oxygen concentration at 75% by a ProOX oxygen controller (BioSpherix). All experimental protocols were reviewed and approved by the Institutional Animal Care and Use Committee of RIKEN CDB and Kobe University Graduate School of Medicine.


The procedures for ISH and immunohistochemistry (IHC) in whole-mount retinas have been described elsewhere (45). For IHC, retinas were incubated with the following primary Abs: polyclonal rabbit anti–type IV collagen (COSMO BIO Co.), monoclonal rat anti–PECAM-1 (clone Mec13.3; BD), polyclonal rabbit anti–neurofilament M (Millipore), and polyclonal rabbit anti-GFP (Invitrogen). The secondary Abs were Alexa Fluor 488–donkey anti-rabbit (Invitrogen) and Cy3–donkey anti-rat (Jackson ImmunoResearch Laboratories Inc.). Nuclear staining was performed using TO-PRO-3 iodide (Invitrogen). For ISH, the templates for cRNA probes (Vegf, 825–1,172 of NM_009505; Plxnd1, 5,184–6,055 of AK129175; Rhoj, 1,203–2,276 of NM_023275) were obtained by reverse transcription of total RNA from P4 ICR mouse retinas with subsequent PCR amplification. The templates for Sema3e RNA probes (46) were gifts from A. Watakabe (National Institute for Basic Biology, Okazaki, Japan). For cryosections, retinas were frozen in OCT compound (Sakura Finetek) after whole-mount ISH and sectioned at a thickness of 10 μm. Images were taken with an LSM510 confocal microscope (Zeiss), or with an Axioplan 2 microscope (Zeiss) equipped with associated software (AxioVision, version 3.1; Zeiss). In combined ISH and IHC, photos of the same fields were taken separately in black and white with an Axioplan 2 microscope. The signals were then colored and merged using Adobe Photoshop CS software.

Intravitreal injections.

PlexinD1-Fc protein was purified using a HiTrap Protein G column (GE Healthcare) from serum-free culture supernatants of FreeStyle 293F cells (Invitrogen) transfected with a plasmid vector expressing the extracellular domain of mouse PlexinD1 (Met1-Gly1266) fused to the Fc fragment of human IgG under control of the CAG promoter (20). Recombinant PlexinD1-Fc, mouse VEGFR1–human Fc (R&D Systems), human Fc (Jackson ImmunoResearch Laboratories Inc.), and human Sema3E (R&D Systems) proteins in sterile buffer were injected into the vitreous humor using glass capillary pipettes with a micromanipulator (Drummond Scientific Co.). In Sema3E-AP binding assays, the retinal cups were removed 2 hours after intravitreal injection of the Sema3E-AP fusion protein, washed, and stained as previously described (14).

Quantitative analysis of the retinal vasculature.

All quantifications were performed in images of flat-mount retinas stained with PECAM-1. The number of endothelial filopodia per 100-μm vessel length, and filopodia lengths were calculated in sprouting vascular fronts photographed at 63× objective using LSM510 confocal image software. The vessel area density in postnatal mouse retinas was calculated in a fixed area (3.63 × 104 μm2) using WinROOF software (version 2.34, Mitani Corp.). The number of extraretinal vascular tufts and the vessel area density in the superficial retina in the OIR model were calculated in thin z-section confocal images (5.3 × 104 μm2) of 4 random areas, and then averaged per retina. For each group, 4 retinas from 4 mice were analyzed. The unvascularized retinal area in the OIR model was calculated in a panoramic view (Supplemental Figures 7 and 8) using WinROOF software. For each group, 4 retinas from 4 mice were analyzed.


Retinal cells dissociated from P8 Tie2GFP Tg mice (47) (The Jackson Laboratory) were separated into GFP-positive ECs and GFP-negative non-ECs by FACSAria (BD). Using total RNA extracted by RNeasy Micro Kit (QIAGEN) and amplified by MessageAmpII aRNA Amplification Kit (Ambion), cRNA was prepared and hybridized onto the Affymetrix oligonucleotide arrays MGU74v2 as described previously (48). Primary data have been deposited in NCBI’s Gene Expression Omnibus and are accessible through GEO series accession number GSE27238. The bioinformatics analyses were performed with the eXintegrator system (49) ( Briefly, probe sets representing small GTPase genes were sorted by their similarity (Euclidean distance) to a specified profile with low or nonexistent signals in non-EC samples and high signals in EC samples. The expression data for the resulting list of genes were then manually inspected to remove genes with expression in the non-EC samples and probe sets with ambiguous identities.

Cell culture and transfection.

HUVECs (Lonza) cultured in Endothelial Growth Medium EGM-2 BulletKit (Lonza) at a density of 5 × 103 cells/cm2 in fibronectin-coated culture slides (BD) were transfected with pCAGGS-EGFP vector together with pCAGGS vector expressing human RhoJ-WT, RhoJ-CA (G30V) (25), or RhoJ-DN (T35N) (25) tagged with c-Myc at the N-terminus, using TransIT-LT1 (Mirus). After 24 hours, cells were fixed with 4% PFA/PBS, incubated with 1% BSA/0.1% Triton-X/PBS, and then stained with anti-GFP Ab (Invitrogen), mouse anti-Myc mAb (clone 9E10; Santa Cruz Biotechnology Inc.), and Alexa Fluor 633–phalloidin (Invitrogen). The specimens were observed with an LSM510 confocal microscope (Zeiss). More information on cell culture experiments is provided in Supplemental Methods.

RNA interference.

Two predesigned duplexes of Stealth Select RNAi siRNAs (HSS126217 and HSS183814, Invitrogen) targeting different sequences of human RhoJ were transfected to cultured HUVECs using Lipofectamine RNAiMAX according to the manufacture’s protocol. Nontargeting siRNA (Stealth RNAi Negative Control Medium GC Duplex, Invitrogen) was used as a negative control. After incubation for 2 days, cells were serum starved with Endothelial Basal Medium EBM-2 (Lonza) containing 0.5% BSA for 12 hours and then stimulated with human Sema3E (500 ng/ml, R&D Systems). After 30 minutes, cells were fixed and stained with Alexa Fluor 488–phalloidin, mouse anti-RhoJ mAb (clone 1E4, Abnova), and TO-PRO-3. Representative data for HSS126217 are presented.

Measurement of RhoJ activity.

RhoJ-GTP levels were measured using the colorimetric G-LISA Cdc42 activation assay (Cytoskeleton Inc.). Briefly, HUVECs cultured at a density of 5 × 103 cells/cm2 in gelatin-coated 60-mm tissue culture dishes (BD) were serum starved for 12 hours, treated with recombinant human VEGF (HumanZyme) and/or human Sema3E (R&D Systems) for 2 minutes, and lysed according to the manufacturer’s protocol. The total protein concentration for each lysate was adjusted to 0.25 mg/ml using binding buffer and incubated in 96-well plates containing the CRIB domain of the human PAK protein, which can bind to RhoJ-GTP (24), linked to the bottom of each well. After sequential incubation with anti-RhoJ mAb (Abnova), HRP-conjugated secondary Ab, and the HRP detection reagent, the amount of RhoJ-GTP was detected by measuring absorbance at 490 nm. The results are expressed relative to the control (cell lysates without VEGF or Sema3E stimulation) and represent an average of 3 experiments.


Statistical analysis was performed with SPSS software (version 10.0J, SPSS Japan Inc.) using 2-tailed, unpaired t tests. P values of less than 0.05 were considered statistically significant.

Supplementary Material

Supplemental data:
Supplemental video 1:
Supplemental video 2:
Supplemental video 3:
Supplemental video 4:


We thank J. Rossant, T.M. Jessell, C.E. Henderson, and R. Wang for mutant mice; L.M. Jakt and S. Kusuhara for microarray analyses; and S. Koyama for morphometric analyses. We are grateful to the Laboratory for Animal Resources and Genetic Engineering at RIKEN CDB for producing R26-Rhoj chimeric mice and housing the mutant mice. This research was funded by the Global Center of Excellence for Education and Research on Signal Transduction Medicine in the Coming Generation and Grants-in-Aid for Young Scientists (no. 22689046) from the Ministry of Education, Culture, Sports, Science, and Technology (MEXT), Japan. A. Uemura is supported by the Takeda Science Foundation, Mitsubishi Pharma Research Foundation, and the Uehara Memorial Foundation. Y. Yoshida is supported by NIH grant R01NS065048.


Conflict of interest: The authors have declared that no conflict of interest exists.

Citation for this article: J Clin Invest. 2011;121(5):1974–1985. doi:10.1172/JCI44900.


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