Search tips
Search criteria 


Logo of plosonePLoS OneView this ArticleSubmit to PLoSGet E-mail AlertsContact UsPublic Library of Science (PLoS)
PLoS One. 2012; 7(8): e43199.
Published online 2012 August 20. doi:  10.1371/journal.pone.0043199
PMCID: PMC3423444

Endothelin B Receptors Contribute to Retinal Ganglion Cell Loss in a Rat Model of Glaucoma

Steven Barnes, Editor


Glaucoma is an optic neuropathy, commonly associated with elevated intraocular pressure (IOP) characterized by optic nerve degeneration, cupping of the optic disc, and loss of retinal ganglion cells which could lead to loss of vision. Endothelin-1 (ET-1) is a 21-amino acid vasoactive peptide that plays a key role in the pathogenesis of glaucoma; however, the receptors mediating these effects have not been defined. In the current study, endothelin B (ETB) receptor expression was assessed in vivo, in the Morrison's ocular hypertension model of glaucoma in rats. Elevation of IOP in Brown Norway rats produced increased expression of ETB receptors in the retina, mainly in retinal ganglion cells (RGCs), nerve fiber layer (NFL), and also in the inner plexiform layer (IPL) and inner nuclear layer (INL). To determine the role of ETB receptors in neurodegeneration, Wistar-Kyoto wild type (WT) and ETB receptor-deficient (KO) rats were subjected to retrograde labeling with Fluoro-Gold (FG), following which IOP was elevated in one eye while the contralateral eye served as control. IOP elevation for 4 weeks in WT rats caused an appreciable loss of RGCs, which was significantly attenuated in KO rats. In addition, degenerative changes in the optic nerve were greatly reduced in KO rats compared to those in WT rats. Taken together, elevated intraocular pressure mediated increase in ETB receptor expression and its activation may contribute to a decrease in RGC survival as seen in glaucoma. These findings raise the possibility of using endothelin receptor antagonists as neuroprotective agents for the treatment of glaucoma.


Glaucoma is an optic neuropathy with a world-wide incidence of nearly 60.5 million patients, characterized by optic nerve degeneration, apoptosis of retinal ganglion cells (RGCs), and corresponding visual field defects, which could lead to blindness [1][3]. Glaucoma and other neurodegenerative diseases have several points of similarities, such as axonal degeneration, selective loss of neuron populations (RGCs selectively undergo apoptosis) [4][8], and glial activation [9]. Elevated intraocular pressure (IOP) is a major risk factor in primary open-angle glaucoma (POAG), which accounts for the majority of glaucoma patients. Apart from its well-known IOP related effects, glaucoma is recognized as a heterogeneous group of multifactorial neurodegenerative diseases with varying etiologies and clinical presentations. Hence, multiple hypotheses have been proposed to explain the pathophysiology of glaucoma, including mechanical stress of elevated IOP, disruption of retrograde transport of neurotrophins [6], ocular ischemia [10][12] glutamate-induced excitotoxicity [13], and oxidative stress [14][16]. Currently, the mainstay of glaucoma treatment is a IOP-lowering drug. However, reduction of IOP can only slow RGC loss and optic nerve damage, but cannot completely prevent further degeneration [17], [18]. Hence, understanding molecular mechanisms contributing to RGC death can lead to the development of more effective treatments for glaucoma patients [19].

Corroborative evidence from several laboratories suggests that endothelin-1 (ET-1), a vasoactive peptide, has neurodegenerative effects in glaucoma [20][22]. However, the exact mechanisms underlying ET-1's actions remain to be elucidated. Studies have shown that ET-1 concentrations are significantly increased in the aqueous humor (AH) of patients with POAG and in animal models of glaucoma [23][25]. Both peribulbar and intravitreal administration of ET-1 has been found to produce axon loss and RGC death [26][30].

ET-1 exerts its functions via binding to two classes of G-protein coupled receptors, namely endothelin A (ETA) and endothelin B (ETB) receptors, both of which are abundantly expressed in various ocular tissues [21], [31], [32]. In animal models of glaucoma, studies have shown that there is an increase in ETB receptor mRNA expression in rat retinas as early as 1 day following IOP elevation and persisted up to 8 weeks of ocular hypertension [33]. Another study [34] demonstrated an increased frequency of ETB receptor immunolocalization in human glaucomatous optic nerves, compared to those of age-matched controls. Previous work from our laboratory suggests that the ETB receptor could be a key mediator of ET-1's neurodegenerative effects following intravitreal administration of ET-1 [30]. The purpose of this study was to analyze ETB receptor expression in the retinas of rats with elevated IOP and to determine if RGC loss is attenuated in ETB receptor-deficient transgenic rats.


Elevation of intraocular pressure produced an upregulation of ETB receptors in rat retinas

Previous studies from our laboratory suggested the involvement of ETB receptors in several cellular pathways contributing to neurodegeneration of RGCs [20], [25], [30]. In the present study, we sought to determine whether there are any changes in the ETB receptor expression in rat retinas following IOP elevation for 2 and 4 weeks. Briefly, Brown Norway rats were used to elevate IOP in one eye while the corresponding contralateral eye served as control. Rats were sacrificed after 2 and 4 weeks of IOP elevation and retina sections were obtained from rat eyes. Immunohistochemical analysis of retinal sections from adult Brown Norway rats showed an increased immunostaining for ETB receptors primarily in the nerve fiber layer (NFL) and ganglion cell layer (GCL) in retinas of rats with IOP elevation for 2 weeks (white arrows, Figure 1B), compared to those of the contralateral control eyes. Increased immunostaining for ETB receptors was also observed in inner plexiform layer (IPL), and outer plexiform layer (OPL) in retinas of rats with IOP elevation for 2 weeks, compared to those of the contralateral control eyes (Fig. 1B). A modest increase in immunostaining for ETB receptors was also seen in the inner nuclear layer (INL) after 2 weeks of IOP elevation. Four weeks of IOP elevation also resulted in an increase in ETB receptor expression primarily in the NFL, GCL, IPL, and OPL in retinas of rats with IOP elevation, as compared to control (Fig. 1D). The increase in ETB receptor expression was similar to that seen after 2 weeks of IOP elevation (Fig. 1B). Based upon values of fluorescence intensities (using the Image J software) obtained from confocal images of retinal sections, there a 2.59 fold increase in ETB receptor immunostaining after 2 weeks of IOP elevation and a 2.52 fold increase after 4 weeks of IOP elevation. Interestingly, robust staining for the ETB receptor was also observed in the INL following 4 weeks of IOP elevation.

Figure 1
IOP elevation produced a marked increase in ETB receptor expression in rat retinas.

To ascertain that an increase in ETB receptor expression occurred in RGCs after IOP elevation, an immunostaining for ETB receptors was performed on retinal sections from Fluoro-Gold (FG) labeled rats. Briefly, retinal ganglion cells of adult male Brown Norway rats were retrogradely labeled with FG, following which IOP was elevated in one eye [35]. After maintaining the rats for 2 weeks following IOP elevation, the animals were sacrificed, retina sections were obtained and immunostained for ETB expression. An increased immunostaining for ETB receptor was observed mainly in retrogradely labeled RGCs in the RGC layer in IOP elevated eyes, compared to the corresponding control eyes (Figure 2B). This provides further confirmation for increased ETB receptor expression in RGCs following IOP elevation in rats.

Figure 2
Increased ETB receptor immunostaining in Fluoro-Gold labeled retinal ganglion cells following IOP elevation in rats.

ETB receptor binding activity was increased in retinas of rats with elevated IOP

Since an increase in ETB proteins was observed by immunostaining in IOP elevated rat retinas, further confirmation was made by receptor binding assays using radiolabeled ET-1. In preliminary experiments 125I-labeled ET-1 was found to bind to rat retinal membrane (3 µg of protein) in a linear pattern. The ETA receptor antagonist, BQ-610, yielded a Ki value of 16.3 nM in competitive binding assays using rat retinal membranes. This experimental Ki is very close to the Ki value (20 nM) provided for BQ-610 by the manufacturer (Peninsula Lab Inc. Belmont, CA, USA). Based on the Ki value, BQ-610 was used at a concentration of 200 nM in the receptor binding assays Three individual binding assays were performed to plot endothelin receptor binding sites in the presence of 0.2–2 nM of 125I-ET-1, 1 µM of unlabeled ET-1 and 200 nM of BQ-610. The number of binding sites, Bmax (fmol/mg), of total endothelin receptors (ETA and ETB receptors) and ETB receptors was calculated for retinas from elevated IOP and contralateral eyes using unweighted linear regression analysis after normalization to the amount of protein by the method of Scatchard [36]. Total specific endothelin receptor binding (Bmax values) in retinal membranes from IOP-elevated eyes increased 2.7-, 1.5- and 1.7-fold respectively (from three independent binding assays) compared to the binding in the contralateral eye (Figure 3B). There was a significant (p<0.05) mean 1.9-fold increase in the total specific endothelin receptor binding activity (Bmax values) in the IOP elevated eyes, compared to the contralateral eyes (Table 1). On the other hand, there was no significant change in the binding affinity (reflected by the Kd values) for the total endothelin binding between control and elevated IOP eyes (Table 2). Specific ETB receptor binding (Bmax values) was increased 4.8-, 3.3- and 2.2-fold in the IOP-elevated eye, compared to the corresponding contralateral eye (Figure 3B). There was a significant (p<0.05) mean 3.3-fold increase in specific ETB receptor binding in IOP elevated eyes, compared to control eyes (Table 1). The Kd values for the specific ETB receptor binding were not significantly different between control and IOP elevated eyes (Table 2). The results indicate that number of endothelin receptors was increased in the retina from IOP-elevated eye, and in particular 125I-ET-1 binding to ETB receptors was even higher in IOP elevated eyes, compared to contralateral eyes.

Figure 3
ETB receptor binding activity was increased in retinas of IOP elevated Brown Norway rats.
Table 1
Bmax values (fmol/mg) for endothelin receptor binding.
Table 2
Kd values (pM) for endothelin receptor binding.

Retinal ganglion cell loss was attenuated in ETB receptor-deficient transgenic rats after 4 weeks of IOP elevation

IOP elevation in the Morrison rat model of glaucoma has been shown to result in a significant increase in TUNEL-positive RGCs, axonal loss, and gliosis [37][39]. However, the key contributors to RGC death are not completely understood. The endothelin family of peptides has recently gained prominence for their neurodegenerative effects in the retina [28], [30], [40]; however, the receptors mediating these effects have not been identified. To determine the involvement of ETB receptors in neurodegenerative effects, RGCs of wild type (WT) and ETB receptor-deficient transgenic rats (KO) were retrogradely labeled with FG, following which IOP elevation was carried out and maintained for 4 weeks (Figure 4A). After sacrificing the animals, retinal flat mounts were obtained and RGC survival was assessed by counting viable RGCs (Figure 4B) in three eccentricities (E1, E2 and E3) within each retinal quadrant (Figure 4C). The loss of RGCs due to IOP elevation was computed by calculating the ratio of RGC counts between left (IOP elevated) and right (control) eye for each eccentricity. The ratio of RGC counts between left and right eye for each eccentricity was then compared between WT and KO rats (Figure 4D). Interestingly, the ratios of RGC counts between left and right eye were significantly higher in KO rats in the first two eccentricities (E1 and E2), compared to those of the WT rats (Figure 4D). The ratio of RGCs counts between left and right eyes was also higher in the third eccentricity of the KO rats; however, it did not attain statistical significance (Figure 4D). These results demonstrate that the ETB receptor may play a causative role in RGC death following elevation of IOP, and blocking this receptor may aid in neuroprotection of RGCs.

Figure 4
RGC loss following IOP elevation was attenuated in KO rats compared to WT rats.

Axonal integrity was maintained in ETB-deficient rats after IOP elevation

Since a significant protection of RGCs was observed in KO rats subjected to IOP elevation, compared to WT rats, optic nerve axonal integrity was assessed in these animals. IOP was elevated in one eye of WT and KO rats, while the corresponding contralateral eye served as control [35]. After IOP elevation, rats were maintained for 4 weeks, sacrificed and optic nerve sections were obtained and stained with paraphenylenediamine (PPD). As seen in Figure 5, an increased staining with PPD was observed in optic nerve sections from IOP elevated WT rats. In addition, disruption of axon bundles, increased gliosis and glial scar formation was seen in the optic nerve sections from WT rats following IOP elevation. In contrast, optic nerve sections from IOP elevated KO rats showed a better preservation of axon morphology (Figure 5). Glial scarring was less prominent in KO rats compared to that seen in WT rats following IOP elevation. Optic nerve grading was done by masked observers essentially according to the method described by Chauhan et al. (2006). Grade 0 was assigned to optic nerves with no damage with all the nerve bundles intact, while grades 3 and 6 correspond to nearly 30% and 60% of mean damage. The analysis indicated that there was no appreciable difference between the integrity of optic nerve between contralateral control eyes of the WT and KO rats (graded 1 to 2). However, the optic nerve sections from IOP elevated KO rat eyes showed lesser damage (graded 2 to 3) compared to optic nerves from the IOP elevated WT rats (graded 3 to 4). These observations suggest that lack of ETB receptor activation could have protective effects on the axons of the optic nerve in addition to preventing RGC loss.

Figure 5
Survival of optic nerve axons in KO rats, compared to WT rats following IOP elevation.

ET-1 treatment produced increased cell death in cultured primary retinal ganglion cells

Primary cultures of RGCs were isolated and were first tested by immunocytochemistry to determine if they express ETB and ETA receptors. Immunostaining for ETB and ETA receptors was observed both in the soma and neurites of cultured primary RGCs (Figure 6A, B). Immunocytochemical analysis of primary RGCs in which the primary antibody was excluded (Blank) showed minimal staining indicating that there was no appreciable non-specific binding of the Alexa647 conjugated secondary antibody (Figure 6C). To determine if endothelin receptor activation could promote death of RGCs, primary RGCs grown on coverslips were treated with two different concentrations of ET-1 (10 nM and 100 nM) or with the ETB receptor agonist, ET-3 (100 nM). Another group of RGCs grown on coverslips that did not undergo any treatment served as controls. Following the treatments, a mixture of green-fluorescent calcein-AM (indicative of intracellular esterase activity of viable cells) and red-fluorescent ethidium homodimer-1 (EtHD) (indicative of loss of plasma membrane integrity of dead cells) was added to assess the viability and death of the cells respectively. As seen in figure 7A, untreated RGCs had good morphology as evidenced by multiple neurites from each cell and forming a network of synaptic connections with neighboring cells. The cells were brightly stained with calcein-AM (green fluorescence) indicating that they were viable. There were also some EtHD stained cells (Mean ± SEM: 27±1.7% of cells) indicative of cell death in the untreated cells, possibly due to loss of trophic support in these cells. In cells treated with 10 nM ET-1 there was a decrease in staining with calcein AM and a withdrawal of neurites from many cells. The number of EtHD stained cells, indicative of cell death significantly increased in the 10 nM ET-1 treated cells (Mean ± SEM: 41±2.7% of cells), compared to the controls. The cell viability was further exacerbated in primary RGCs when treated with 100 nM ET-1. These cells exhibited fewer processes, compared to the 10 nM treatment, and nuclei were found to be more condensed indicative of apoptotic changes (Figure 7A). Moreover, RGCs treated with 100 nM ET-1 showed significantly higher EtHD staining (Mean ± SEM: 43±4.2% of cells), compared to untreated control cells (Figure 7B). Primary RGCs treated with the ETB receptor agonist, ET-3, demonstrated almost complete withdrawal of neurites and also showed significantly higher number of EtHD staining indicative of cell death, compared to controls (Mean ± SEM: 43±2.9% of cells) (Figure 7B). These results suggest that ET-1 acting predominantly through the ETB receptor promotes cell death of RGCs.

Figure 6
Immunocytochemical analysis of endothelin receptor expression in primary rat retinal ganglion cells (RGCs).
Figure 7
Live-dead assay of primary RGCs treated with endothelins.

ET-1 treatment promoted cell death via apoptosis in primary retinal ganglion cells

Since ET-1 treatment produced increased cell death of primary retinal ganglion cells, further experiments were carried out to ascertain if this occurred through an apoptotic mechanism. To test this, primary RGCs were isolated from post natal day 3–7 rat pups, seeded on 12 mm coverslips and allowed to attach and grow for 1 week. The RGCs were either untreated or treated with ET-1 (10 nM), ET-1 (100 nM) or ET-3 (100 nM) for 24 hr. After the treatments, cells were fixed with 4% paraformaldehyde for 25 min at 4°C and TUNEL assays were carried out to detect apoptotic cell death using a commercially available kit from Promega (Madison, WI, USA) as per the manufacturer's instructions. As seen in Figure S1, RGCs treated with a reaction mix in which the TdT enzyme was excluded (negative control) showed no staining whereas cells treated with DNAse I to introduce artificial strand breaks (positive control) yielded a robust TUNEL positive reaction, ensuring the validity of the TUNEL assay. Untreated RGCs showed minimal staining for TUNEL positive cells, indicating that there was no appreciable apoptotic cell death in the untreated RGCs (Figure 8). However, in both 10 nM and 100 nM ET-1 treatment increased TUNEL labeling was observed, indicative of apoptosis (Figure 8). The most intense TUNEL labeling was observed in primary RGCs treated with the ETB receptor agonist, ET-3, suggesting that the ETB receptor could be a key mediator of apoptosis in RGCs (Figure 8).

Figure 8
TUNEL assay of primary RGCs treated with endothelins.


An accumulating body of evidence suggests the involvement of ET-1 [20], [21], [41][43] and ETB receptors [25], [30], [33], [34], [42], [44][46] in the pathogenesis of glaucoma, however a causal link of ETB receptors to neurodegeneration has not been clearly established.

The endothelin family is comprised of three endothelin isoforms, namely ET-1, ET-2, and ET-3, each of which is encoded by different genes [47], [48]. ET-1 is the most studied isoform, which is constitutively synthesized and secreted from several tissues. Originally purified and characterized from vascular endothelial cells [49], ET-1 has been shown to be present in several tissues and organs including the eye [50][52] and brain [53], [54]. The normal physiological role of ET-1 in the central nervous system remains to be understood. However, studies have demonstrated that ET-1 is a key player in various neurodegenerative conditions, including Alzheimer's disease, retinal degeneration and glaucoma [22], [40], [55], [56]. In Parkinson's disease, the Parkin-associated endothelin receptor-like receptor (Pael-R) has been shown to induce unfolded protein response (UPR)-mediated cell death [57]. Nevertheless, the detailed mechanisms underlying ET-1's neurodegenerative effects remain to be elucidated.

ET-1 exerts its functions via binding to two classes of G-protein coupled receptors, ETA and ETB [21], [31], [32]. The two receptors have different affinities for the different endothelin peptides. The ETA receptor has equal affinity for ET-1 and ET-2 peptides, but much lower affinity for ET-3 (ETA: ET-1 = ET-2 » ET-3), while the ETB receptor has equal affinity for all the three endothelin peptides (ETB: ET-1 = ET-2 = ET-3). Thus, ET-3 could be used as an ETB receptor agonist. Clinical studies have found increased levels of ET-1 in aqueous humor of primary open angle glaucoma patients [58] and increased circulating levels of ET-1 in normal tension glaucoma patients [59]. ET-1 concentrations were also found to be elevated in exfoliation syndrome (the production and progressive accumulation of a fibrillar extracellular material in many ocular tissues) [60], [61]. ETA-like receptor binding sites have been identified in the retina and choroidal blood vessels [31]. In contrast, ETB-like receptor-binding sites were primarily found in the neural and glial components of the retina [32], [62]. Studies have demonstrated that primary cultures of human trabecular meshwork, ciliary muscle, and ciliary nonpigmented epithelial cells predominately express the ETA receptor [62].

Since ETB receptor expression increases at very early time points of IOP elevation (when no appreciable loss of RGCs occurs) [33], it could play a causative role in neurodegeneration in glaucoma. Interestingly, we found a profound increase in ETB receptor expression in the nerve fiber layer (NFL) and ganglion cell layer (GCL) in retinas of rats with IOP elevation for 2 weeks, compared to those of the contralateral control eye (Fig. 1B) and this elevation in ETB receptor expression was maintained up to 4 weeks of IOP elevation. Since RGCs are located in the GCL along with displaced amacrine cells [63][65], it is important to distinguish between these two cell populations to conclude that changes in ETB receptor expression occur primarily in RGCs in IOP elevated eyes. An increased staining of ETB receptors was observed mainly in the FG labeled RGCs in the RGC layer after IOP elevation for 2 weeks (Figure 2B). We also observed an increase in the expression of ETB receptors in the inner plexiform layer (IPL) and outer plexiform layer (OPL) in retinas of rats with IOP elevation for 2 weeks, in comparison to contralateral control eye (Fig. 1B). It is known that IPL is the layer where the bipolar cell axons form synapses with dendrites of the ganglion and amacrine cells, whereas OPL contains projections of rods and cones [66]. Interestingly, increased staining for ETB receptors was observed in the inner nuclear layer (INL) following 4 weeks of IOP elevation INL, which is composed the cell bodies of the bipolar, horizontal, and amacrine cells (Figure 1D). The significance of upregulation of ETB receptors in these retinal layers is currently unclear, however these cell types do not undergo pathological changes in glaucoma.

Receptor-binding assays using 125I-ET-1 showed a preferential upregulation of ETB receptors in the retina following IOP elevation. A significant increase in the Bmax values (indicative of number of receptor binding sites) for ETB receptor binding was observed without a significant increase in the corresponding Kd values (indicative of receptor affinity), which is a classic pharmacological measure of upregulation of receptor expression. ETB receptors function as clearance receptors and play a critical role in maintaining normal levels of ET-1 [67], [68]. It is possible that expression of ETB receptors is increased in response to elevation of ET-1 concentrations following IOP elevation. Increased expression of ETB receptors was also detected at the level of the optic nerve head in animal models, as well as in glaucoma patients [25], [30], [34]. In animal models of photoreceptor degeneration, another member of the endothelin family, ET-2, was found to be elevated and accompanied by more than 10-fold increase in ETB expression primarily in the glial cells in the retina [40].

In glaucoma, RGCs are selectively lost via apoptosis [7], [69][73], while other retinal neurons are largely unaffected. However, the key contributors to RGC death have not been completely identified. To assess RGC viability in vivo, we used retrograde labeling with FG, which has been shown to label 98.4% and 97.8% of the RGCs in albino and pigmented rats, respectively [74]. Using this method followed by IOP elevation, it was found that four weeks of IOP elevation in WT rats produced a significant loss of RGCs. In contrast, loss of RGCs was significantly attenuated (p<0.05) in the first two eccentricities in retinas of KO rats, compared to those of WT rats. Apart from RGCs, neuroprotective effects were also observed in the axons of KO rats in comparison to WT rats following IOP elevation. Considering the robust neuroprotection observed in KO rats, it is possible that ETB receptor activation in multiple cell types (including lamina cribrosa, RGCs and optic nerve head astrocytes) may be contributing to neurodegeneration in glaucoma. Thus, blocking ETB receptors could have additive neuroprotective effects due to the involvement of ETB receptors in pathological changes in several tissues in glaucoma.

Using primary RGCs, it was found that ET-1 treatment at two different concentrations (10 and 100 nM) produced a significant increase in cell death, suggesting that ET-1 acting through its receptors produces neurodegenerative effects. Since ET-3, an ETB receptor agonist, produced a similar extent of cell death as seen with ET-1 (which acts on both ETA and ETB receptors), it is possible most of endothelin-1 mediated degenerative effects on RGCs occur through the ETB receptors. Using the TUNEL assay, it was found that the mode of cell death by ET-1 treatment was via apoptosis in primary RGCs. The ETB receptors appeared to play a key role in apoptotic cell death of RGCs since the most intense TUNEL labeling was observed in primary RGCs treated with an ETB receptor agonist (ET-3) (Figure 8). In a recent study, bosentan treatment (which blocks both ETA and ETB receptors) was shown to protect against axonal degeneration in the DBA/2J mouse model of glaucoma, suggesting that some of the degenerative effects could also occur through the ETA receptor [75].

In conclusion, we have found that upregulation of ETB receptors in RGCs occurs at early stages in the Morrison's ocular hypertension rodent model of glaucoma, and may contribute to the death of RGCs. Endothelin receptor antagonists could be promising candidates for neuroprotection in glaucoma.

Materials and Methods


All animal experiments were performed in accordance with the Association for Research in Vision and Ophthalmology (ARVO) policy on the Use of Animals in Vision Research, and all protocols were reviewed and approved by the institutional animal care and use committee (IACUC) at the University of North Texas Health Science Center. Adult male retired breeder Brown Norway (Rattus norvegicus) rats (200–350 g) were purchased from Charles River (Wilmington, MA). Wistar-Kyoto ETB receptor-deficient transgenic rats (KO) (a kind gift from Dr. Masashi Yanagisawa, UT Southwestern Medical Center, Dallas, Texas) were maintained in the vivarium at the UNT Health Science Center. The rats were rescued transgenic ETB-deficient spotting lethal (TGETBsl/sl) rats. The parental heterozygous spotting lethal strain carries a naturally occurring deletion in the first exon of the ETB receptor gene that completely abrogates expression of a functional ETB receptor. Deletion of the ETB receptor in rats is lethal beyond the first few weeks after birth due to aganglionic intestinal obstruction. However, the ETB receptor-deficient transgenic rats used in this study had been rescued by tissue-specific expression of the ETB receptor in the intestine, mediated by the dopamine-β-hydroxylase promoter linked to a functional ETB transgene, which directs ETB expression specifically to the intestine. This allows for normal development of the enteric nervous system; thus, preventing neonatal lethality in these ETB-deficient rats [76]. Heterozygous breeding pairs were used to produce offsprings typically with a Mendelian ratio of genotypes. We performed routine genotyping of rat pups to ensure the genotypes of the WT and KO rats that were used in these studies. Rats were maintained under constant low illumination (90 lux).

Retrograde labeling with Fluoro-Gold (FG)

Retrograde labeling of RGCs was carried out in WT and KO rats as described earlier [77]. The animals were anesthetized with intraperitoneal injection (i.p.) of an anesthesia cocktail comprising of 50 mg/ml ketamine, 5 mg/ml xylazine and 1 mg/ml acepromazine (100 µl/100 g body weight) and placed into a stereotaxic frame (Tujunga, CA, USA) to secure the cranium. Double injections of FG (Denver, CO, USA), were carried out using two sets of stereotaxic coordinates: (i) anterior posterior (AP) = 5.8, ML = +1.3, DV = 3.5 and (ii) AP = 5.8, ML = −1.3, DV = 3.5 from the bregma. For each injection, approximately 3 µl of FG (2% solution in isotonic saline) were injected using a 10 µl Hamilton syringe (Reno, NV, USA) at a rate of 1 µl/min. Following recovery for 2 weeks, IOP was elevated in one eye of each rat by injection of hypertonic saline through episcleral veins [35].

Morrison's ocular hypertension model of glaucoma in rats

The procedure of Morrison et al. (1997) was used to elevate IOP in rats [35]. Initial studies were carried out in male Brown Norway retired breeder rats to study the effect of elevated IOP on expression of ETB receptors in the retina. To test the role of ETB receptors in neurodegeneration, wild type and ETB receptor-deficient transgenic rats were used after IOP elevation. Animals were maintained on a reduced constant light environment of 90 lux for a minimum of 3 days prior to surgery for elevating IOP. Daily IOP measurements using a Tonolab tonometer (Icare Finland Oy, Espoo, Finland), conducted on the conscious animals after slight sedation with intramuscular (i.m.) administration of acepromazine. On the day of the surgery, animals were anesthetized with an i.p. injection of a standard rat cocktail consisting of ketamine, xylazine, and acepromazine. One eye of each animal was injected with 1.8 M hypertonic saline via an episcleral vein, while the contralateral eye served as a control. A micro glass needle was inserted into the episcleral vein and approximately 50 µl of hypertonic saline was injected with a force sufficient to blanch the aqueous plexus. This procedure produces scarring of the trabecular meshwork with a resultant rise in IOP and damage to the optic nerve [35]. The rats were sacrificed by overdose with pentobarbital (administered first intraperitoneal and then intracardial) at two different time points (2 and 4 weeks) following IOP elevation.

IOP measurements

IOP was measured in conscious animals using Tonolab tonometer (iCare, Finland). Rats were slightly sedated by an intramuscular injection of acepromazine (2 mg/kg) and IOP measurements were taken 2 to 5 min after the injection. During each IOP measurement session, ten average readings from control and IOP-elevated eyes were obtained. A plot of mean IOP versus time was carried out and IOP exposure was calculated as the number of mmHg days by performing a separate “area-under the curve” (AUC) integration of IOP over the days of exposure for the treated and control eye in each rat [78]. The integral IOP value of the control eye was subtracted from the integral value of the IOP-elevated eye to give the “IOP-integral difference” which was expressed as mmHg days.

Quantification of RGC survival

Retrograde labeling of retinal ganglion cells using FG was carried out in rats as described by Husak et al. (2000). Two weeks following retrograde labeling, IOP was elevated in the left eye, while the right eye served as the contralateral control eye. After IOP elevation for 4 weeks, rats were sacrificed using intraperitoneal injection of pentobarbital (120 mg/kg), and the orientation of each eye was marked. Eyes were enucleated and immersion-fixed in 4% paraformaldehyde (PFA) (Phillipsburg, NJ, USA) in 0.1 M sodium phosphate, pH 7.2, for 3 h at room temperature. The retinas were dissected and flat-mounted in fluorosave reagent (Calbiochem, USA). Fluorescent images of the retinal flat mounts were taken using a Zeiss LSM 510 META confocal microscope.

FG-labeled cells were manually counted by a blinded observer using fluorescent images obtained from the confocal microscope. Each retina was divided into four quadrants: superior, inferior, nasal, and temporal. Six pictures were taken at 40× magnification in each retinal quadrant. Briefly, the number of RGCs was counted in a blinded manner in 6 areas per retinal quadrant at three different eccentricities (E1, E2 and E3) located at 2/6, 4/6, and 5/6 of the radius of the retina from the optic nerve head respectively (Figure 4C). A total of 24 pictures were taken from each retina. The number of FG-labeled RGC was counted as relatively round somata with dendritic processes from a slide-projected image with 0.37 to 0.53 mm2 area of the retina. The spindle-shaped, FG-positive microglia could be easily recognized from these photographs and were not counted. RGC survival was expressed as a ratio of the counts in the elevated IOP eye to that of the contralateral control eye, for the same eccentricity.


Retinal sections from Brown Norway rats were subjected to immunohistochemical detection of ETB receptor expression essentially as described by Krishnamoorthy et al. [30]. Briefly, five-micron saggital retinal sections through the optic nerve head were de-paraffinised in xylene (Fisher Scientific, NJ, USA), re-hydrated using a descending series of ethanol washes. Following permeabilization with 0.1% Triton X-100 and blocking with 5% Donkey serum and 5% BSA in PBS, retinal sections were treated with primary antibodies: custom made rabbit anti-ETB (Antibody Research Corporation, St. Charles, MO) diluted 1[ratio]200 (7.5 µg/ml), and incubated for 1 h at room temperature. Secondary incubation for 1 hr was carried out with a 1[ratio] 1000 dilution of the appropriate secondary antibody conjugated with Alexa 488 (Molecular Probes, Eugene, OR). Retinal sections in which the primary antibody incubation was excluded served as blanks and were used to assess non-specific staining by the secondary antibody. Fluorescence images were taken in a Zeiss LSM 510 META confocal microscope.

Receptor Binding Assays

IOP was elevated in the left eye of Brown Norway rats by the method of Morrison et al. (1997), while the corresponding right eye served as contralateral control. After maintaining the rats with elevated IOP for 2 weeks, they were sacrificed and retinas were isolated form left and right eyes. The retinas were homogenized in a solution of 1× TBS (50 mM Tris.HCl, pH 7.4 and 150 mM NaCl) containing protease inhibitors and plasma membrane fractions were isolated by centrifugation at 100, 000 g.

Approximately 3 µg of membrane protein from rat retinas were used for each binding reaction. 125I-ET-1 (NEN Life Science Products Inc., Boston, MA, USA) binding was performed in polypropylene tubes in a total assay volume of 90 µl containing 30 µl of 125I-ET-1 (ranged from 0.2 to 2 nM), 30 µl of membrane fraction and 30 µl of competition reagent (either cold ET-1 or ETA receptor antagonist) or buffer at 37°C for 1 hr. Binding was terminated by adding 5 ml of cold wash buffer (10 mM Tris.HCl pH 7.4 containing 150 mM NaCl) and binding solution was rapidly vacuum filtered through glass fiber filters (No. 30, Schleicher and Schuell Keene, NH, USA). Filters were washed twice with 5 ml of wash buffer and the bound radioactivity was quantitated in a gamma counter. Non-specific binding was assessed by determining filter-bound radioactivity in the presence of 1 µM unlabeled ET-1 (Bachem, Torrance, CA, USA) after addition of 125I-ET-1. The binding of ETA receptor was determined by measuring the decrease in binding in the presence of 200 nM of BQ-610 (ETA receptor antagonist) (Peninsula Lab Inc. Belmont, CA, USA). ETB receptor binding was defined as the total specific 125I-ET-1 binding minus the amount of ETA receptor binding. Estimates of maximum number of binding sites (Bmax) were obtained using unweighted linear regression analysis of data transformed by the method of Scatchard [36].

Live-Dead Assay for primary RGC viability

Primary cultures of rat retinal ganglion cells were prepared using a two-step panning procedure [79]. Briefly, post-natal 3–7 day old Sprague Dawley rat pups (30 pups from 3 litters) (Charler River, Wilmington, MA) were euthanized, and the retinas were placed in 4.5 units/mL of papain solution (Worthington, Lakewood, NJ) to dissociate the tissue. This was followed by incubation of cells for 10 min with a rabbit anti-macrophage antibody (Cedarlane, Burlington, Onatario, Canada). After that cell suspensions were incubated in a 150-mm Petri dish coated with a goat anti-rabbit IgG (H+L chain) antibody (Jackson ImmunoResearch, West Grove, PA) for 30 minutes. Cells that did not adhere to the 150-mm dish were then transferred to a 100-mm dish coated with anti-Thy1.1 antibody (from hybridoma T11D7; American Type Culture Collection, Rockville, MD) for 45 minutes. Cells were then trypsinized off (1250 units/mL) (Sigma-Aldrich, St. Louis, MO) the petri dish and plated on coverslips coated with mouse-laminin (Trevigen Inc., Gaithersburg, MD). Then, cells were cultured in a serum free defined media containing BDNF (50 ng/mL) (Peprotech, Rocky Hill, NJ), CNTF (10 ng/mL) (Peprotech, Rocky Hill, NJ), and forskolin (5 ng/mL) (Sigma-Aldrich, St. Louis, MO). Cells were incubated at 37°C in a humidified atmosphere of 10% CO2 and 90% air.

After 1 week in culture, primary RGCs were viable and showed good neurite outgrowth. Primary RGCs grown on coverslips were either untreated (control) or were treated with ET-1(10 nM and 100 nM) or ET-3 (100 nM) for 24 hr. The cells were treated with a mixture of green-fluorescent calcein-AM (to indicate intracellular esterase activity of living cells) and red-fluorescent ethidium homodimer-1 (EtHD) (indicative of dead cells) was added to assess the viability of the cells (Live/Dead® Viability/Cytotoxicity Kit, Eugene, OR, USA). Eight images were taken for each treatment condition, in a Zeiss LSM 510 META confocal microscope and the number of viable and dead cells was counted using the image J software. The number of dead cells were expressed as a percentage of total cells in each field of view and mean values of percent of dead cells for each treatment condition was calculated. Statistical analyses were performed by One Way ANOVA to determine if there was a significant increase in cell death in various treatment groups in comparison to the untreated control group.

Paraphenylenediamine (PPD) staining

IOP elevation was carried out in WT and KO rats [35]. The rats were maintained for 4 weeks after IOP elevation, following which they were sacrificed, eyes enucleated and optic nerves were excised 2 mm posterior to the globe. The optic nerves were fixed with 2% paraformaldehyde, 2.5% glutaraldehyde in 0.1 M sodium cacodylate buffer for 3 hrs at room temperature. After osmification and embedding in epon, optic nerve cross sections were obtained and stained with 1% paraphenylenediamine for 10 min at room temperature by a modification of a published protocol [80]. Images were taken in a Zeiss LSM 510 META confocal microscope. The images were graded in a blinded manner by five individuals giving a score ranging from 0 to 9 by a modification of the method [81]. The grades assigned to each treatment group were compared to determine if there were neuroprotective/neurodegenerative changes between the different groups.

TUNEL assay for detection of apoptosis

Primary RGCs were isolated from postnatal day 3–7 rat pups using a two step panning procedure (78) and seeded on 12 mm coverslips. The cells were allowed to attach and grow for 1 week till they displayed good neurite outgrowth. The RGCs were either untreated or treated with ET-1 (10 nM), ET-1 (100 nM) or ET-3 (100 nM) for 24 hr. Following treatments, the RGCs on coverslips were fixed with 4% formaldehyde in PBS for 25 min at 4°C. TUNEL assays were carried out using the DeadEnd Fluorometric TUNEL System (Promega, Madison, WI) by the manufacturer's instructions. Briefly, the cells were permeabilized in 0.2% Triton X-100 in PBS for 5 min followed by two washes with PBS. A negative control reaction was carried out by incubating one coverslip of RGCs with fluorescein-12-dUTP in the absence of TdT enzyme. Another coverslip was treated with DNase I enzyme to introduce DNA cleavage prior to the incubation with the reaction mix. The labeling reaction was carried out by incubating with a mixture of fluorescein-12-dUTP and terminal deoxynucleotidyl transferase (TdT) at for 60 min at 37°C. Following the incubation, the cells were washed with PBS and incubated with 4′ 6 Diamidino-phenylindole dichloride (DAPI) to stain nuclei. The TUNEL positive cells were detected by incorporation of fluorescein and fluorescent images were taken in an EVoS microscope.

Supporting Information

Figure S1

Experimental controls for TUNEL assay of primary RGCs. Primary RGCs were either untreated (top horizontal panel) or treated with DNAse I as a positive control (middle horizontal panel). TUNEL assay was carried out using a combination of terminal deoxynucleotidyl transferase (TdT) and fluorescein-12-dUTP. Another set of RGCs were subjected to the negative control reaction by treatment with fluorescein-12-dUTP alone, with the exclusion of TdT (lower horizontal panel). The left vertical panel (TUNEL) indicates fluorescent images from cells incorporating fluorescein-12-dUTP indicative of apoptosis. The right vertical panel (DAPI) shows stained nuclei using DAPI. Scale bar indicates 400 µm.



The authors thank Dr. Thomas Yorio for several useful discussions, insightful comments and suggestions on the manuscript. The technical assistance of Ms. Michelle Taylor in receptor binding assays is gratefully acknowledged. We also thank Mr. Yong Park for help with the primary culture of retinal ganglion cells.

Funding Statement

This work was supported by a National Glaucoma Research grant from the American Health Assistance Foundation (AHAF) and by funding from National Eye Institute (1RO1EY019952) to RRK. The funders had no role in study design, data collection and analysis, decision to publish, or preparation of the manuscript.


1. Quigley HA (1996) Number of people with glaucoma worldwide. Br J Ophthalmol 80: 389–393 [PMC free article] [PubMed]
2. Quigley HA, Broman AT (2006) The number of people with glaucoma worldwide in 2010 and 2020. Br J Ophthalmol 90: 262–267 [PMC free article] [PubMed]
3. Gupta N, Yucel YH (2007) Glaucoma as a neurodegenerative disease. Curr Opin Ophthalmol 18: 110–114 [PubMed]
4. Quigley HA, Addicks EM (1980) Chronic experimental glaucoma in primates. II. Effect of extended intraocular pressure elevation on optic nerve head and axonal transport. Invest Ophthalmol Vis Sci 19: 137–152 [PubMed]
5. Quigley HA, Addicks EM, Green WR (1982) Optic nerve damage in human glaucoma. III. Quantitative correlation of nerve fiber loss and visual field defect in glaucoma, ischemic neuropathy, papilledema, and toxic neuropathy. Arch Ophthalmol 100: 135–146 [PubMed]
6. Quigley HA (1995) Ganglion cell death in glaucoma: pathology recapitulates ontogeny. Aust N Z J Ophthalmol 23: 85–91 [PubMed]
7. Quigley HA, Nickells RW, Kerrigan LA, Pease ME, Thibault DJ, et al. (1995) Retinal ganglion cell death in experimental glaucoma and after axotomy occurs by apoptosis. Invest Ophthalmol Vis Sci 36: 774–786 [PubMed]
8. Kerrigan LA, Zack DJ, Quigley HA, Smith SD, Pease ME (1997) TUNEL-positive ganglion cells in human primary open-angle glaucoma. Arch Ophthalmol 115: 1031–1035 [PubMed]
9. Varela HJ, Hernandez MR (1997) Astrocyte responses in human optic nerve head with primary open-angle glaucoma. J Glaucoma 6: 303–313 [PubMed]
10. Begg IS, Drance SM (1971) Progress of the glaucomatous process related to recurrent ischaemic changes at the optic disc. Exp Eye Res 11: 141. [PubMed]
11. Hayreh SS (1971) Posterior ciliary arterial occlusive disorders. Trans Ophthalmol Soc U K 91: 291–303 [PubMed]
12. Cioffi GA (1996) Care guidelines and optic nerve assessment. J Glaucoma 5: A12. [PubMed]
13. Vorwerk CK, Lipton SA, Zurakowski D, Hyman BT, Sabel BA, et al. (1996) Chronic low-dose glutamate is toxic to retinal ganglion cells. Toxicity blocked by memantine. Invest Ophthalmol Vis Sci 37: 1618–1624 [PubMed]
14. Levin LA (1999) Direct and indirect approaches to neuroprotective therapy of glaucomatous optic neuropathy. Surv Ophthalmol 43 Suppl 1: S98–101 [PubMed]
15. Osborne NN (2008) Pathogenesis of ganglion “cell death” in glaucoma and neuroprotection: focus on ganglion cell axonal mitochondria. Prog Brain Res 173: 339–352 [PubMed]
16. Kong GY, Van Bergen NJ, Trounce IA, Crowston JG (2009) Mitochondrial dysfunction and glaucoma. J Glaucoma 18: 93–100 [PubMed]
17. Cockburn DM (1983) Does reduction of intraocular pressure (IOP) prevent visual field loss in glaucoma? Am J Optom Physiol Opt 60: 705–711 [PubMed]
18. Chauhan BC, Drance SM (1992) The relationship between intraocular pressure and visual field progression in glaucoma. Graefes Arch Clin Exp Ophthalmol 230: 521–526 [PubMed]
19. Almasieh M, Wilson AM, Morquette B, Cueva Vargas JL, Di Polo A (2012) The molecular basis of retinal ganglion cell death in glaucoma. Prog Retin Eye Res 31: 152–181 [PubMed]
20. Yorio T, Krishnamoorthy R, Prasanna G (2002) Endothelin: is it a contributor to glaucoma pathophysiology? J Glaucoma 11: 259–270 [PubMed]
21. Chauhan BC (2008) Endothelin and its potential role in glaucoma. Can J Ophthalmol 43: 356–360 [PubMed]
22. Rosenthal R, Fromm M (2011) Endothelin antagonism as an active principle for glaucoma therapy. Br J Pharmacol 162: 806–816 [PMC free article] [PubMed]
23. Tezel G, Kass MA, Kolker AE, Becker B, Wax MB (1997) Plasma and aqueous humor endothelin levels in primary open-angle glaucoma. J Glaucoma 6: 83–89 [PubMed]
24. Kallberg ME, Brooks DE, Garcia-Sanchez GA, Komaromy AM, Szabo NJ, et al. (2002) Endothelin 1 levels in the aqueous humor of dogs with glaucoma. J Glaucoma 11: 105–109 [PubMed]
25. Prasanna G, Hulet C, Desai D, Krishnamoorthy RR, Narayan S, et al. (2005) Effect of elevated intraocular pressure on endothelin-1 in a rat model of glaucoma. Pharmacol Res 51: 41–50 [PubMed]
26. Orgul S, Cioffi GA, Wilson DJ, Bacon DR, Van Buskirk EM (1996) An endothelin-1 induced model of optic nerve ischemia in the rabbit. Invest Ophthalmol Vis Sci 37: 1860–1869 [PubMed]
27. Cioffi GA, Sullivan P (1999) The effect of chronic ischemia on the primate optic nerve. Eur J Ophthalmol 9 Suppl 1: S34–36 [PubMed]
28. Chauhan BC, LeVatte TL, Jollimore CA, Yu PK, Reitsamer HA, et al. (2004) Model of endothelin-1-induced chronic optic neuropathy in rat. Invest Ophthalmol Vis Sci 45: 144–152 [PubMed]
29. Lau J, Dang M, Hockmann K, Ball AK (2006) Effects of acute delivery of endothelin-1 on retinal ganglion cell loss in the rat. Exp Eye Res 82: 132–145 [PubMed]
30. Krishnamoorthy RR, Rao VR, Dauphin R, Prasanna G, Johnson C, et al. (2008) Role of the ETB receptor in retinal ganglion cell death in glaucoma. Can J Physiol Pharmacol 86: 380–393 [PubMed]
31. MacCumber MW, D'Anna SA (1994) Endothelin receptor-binding subtypes in the human retina and choroid. Arch Ophthalmol 112: 1231–1235 [PubMed]
32. Stitt AW, Chakravarthy U, Gardiner TA, Archer DB (1996) Endothelin-like immunoreactivity and receptor binding in the choroid and retina. Curr Eye Res 15: 111–117 [PubMed]
33. Yang Z, Quigley HA, Pease ME, Yang Y, Qian J, et al. (2007) Changes in gene expression in experimental glaucoma and optic nerve transection: the equilibrium between protective and detrimental mechanisms. Invest Ophthalmol Vis Sci 48: 5539–5548 [PubMed]
34. Wang L, Fortune B, Cull G, Dong J, Cioffi GA (2006) Endothelin B receptor in human glaucoma and experimentally induced optic nerve damage. Arch Ophthalmol 124: 717–724 [PubMed]
35. Morrison JC, Moore CG, Deppmeier LM, Gold BG, Meshul CK, et al. (1997) A rat model of chronic pressure-induced optic nerve damage. Exp Eye Res 64: 85–96 [PubMed]
36. Scatchard G (1949) Equilibrium in non-electrolyte mixtures. Chem Rev 44: 7–35 [PubMed]
37. McKinnon SJ, Lehman DM, Kerrigan-Baumrind LA, Merges CA, Pease ME, et al. (2002) Caspase activation and amyloid precursor protein cleavage in rat ocular hypertension. Invest Ophthalmol Vis Sci 43: 1077–1087 [PubMed]
38. Schlamp CL, Johnson EC, Li Y, Morrison JC, Nickells RW (2001) Changes in Thy1 gene expression associated with damaged retinal ganglion cells. Mol Vis 7: 192–201 [PubMed]
39. Chauhan BC, Pan J, Archibald ML, LeVatte TL, Kelly ME, et al. (2002) Effect of intraocular pressure on optic disc topography, electroretinography, and axonal loss in a chronic pressure-induced rat model of optic nerve damage. Invest Ophthalmol Vis Sci 43: 2969–2976 [PubMed]
40. Rattner A, Nathans J (2005) The genomic response to retinal disease and injury: evidence for endothelin signaling from photoreceptors to glia. J Neurosci 25: 4540–4549 [PubMed]
41. Prasanna G, Narayan S, Krishnamoorthy RR, Yorio T (2003) Eyeing endothelins: a cellular perspective. Mol Cell Biochem 253: 71–88 [PubMed]
42. Rao VR, Krishnamoorthy RR, Yorio T (2007) Endothelin-1, endothelin A and B receptor expression and their pharmacological properties in GFAP negative human lamina cribrosa cells. Exp Eye Res 84: 1115–1124 [PubMed]
43. Prasanna G, Krishnamoorthy R, Yorio T (2011) Endothelin, astrocytes and glaucoma. Exp Eye Res 93: 170–177 [PMC free article] [PubMed]
44. Wang X, LeVatte TL, Archibald ML, Chauhan BC (2009) Increase in endothelin B receptor expression in optic nerve astrocytes in endothelin-1 induced chronic experimental optic neuropathy. Exp Eye Res 88: 378–385 [PubMed]
45. Resch H, Karl K, Weigert G, Wolzt M, Hommer A, et al. (2009) Effect of dual endothelin receptor blockade on ocular blood flow in patients with glaucoma and healthy subjects. Invest Ophthalmol Vis Sci 50: 358–363 [PubMed]
46. Murphy JA, Archibald ML, Chauhan BC (2010) The role of endothelin-1 and its receptors in optic nerve head astrocyte proliferation. Br J Ophthalmol 94: 1233–1238 [PubMed]
47. Rubanyi GM, Polokoff MA (1994) Endothelins: molecular biology, biochemistry, pharmacology, physiology, and pathophysiology. Pharmacol Rev 46: 325–415 [PubMed]
48. Good TJ, Kahook MY (2010) The role of endothelin in the pathophysiology of glaucoma. Expert Opin Ther Targets 14: 647–654 [PubMed]
49. Yanagisawa M, Kurihara H, Kimura S, Tomobe Y, Kobayashi M, et al. (1988) A novel potent vasoconstrictor peptide produced by vascular endothelial cells. Nature 332: 411–415 [PubMed]
50. MacCumber MW, Ross CA, Glaser BM, Snyder SH (1989) Endothelin: visualization of mRNAs by in situ hybridization provides evidence for local action. Proc Natl Acad Sci U S A 86: 7285–7289 [PubMed]
51. MacCumber MW, Jampel HD, Snyder SH (1991) Ocular effects of the endothelins. Abundant peptides in the eye. Arch Ophthalmol 109: 705–709 [PubMed]
52. Wollensak G, Schaefer HE, Ihling C (1998) An immunohistochemical study of endothelin-1 in the human eye. Curr Eye Res 17: 541–545 [PubMed]
53. Lee ME, de la Monte SM, Ng SC, Bloch KD, Quertermous T (1990) Expression of the potent vasoconstrictor endothelin in the human central nervous system. J Clin Invest 86: 141–147 [PMC free article] [PubMed]
54. MacCumber MW, Ross CA, Snyder SH (1990) Endothelin in brain: receptors, mitogenesis, and biosynthesis in glial cells. Proc Natl Acad Sci U S A 87: 2359–2363 [PubMed]
55. Nie XJ, Olsson Y (1996) Endothelin peptides in brain diseases. Rev Neurosci 7: 177–186 [PubMed]
56. Torbidoni V, Iribarne M, Ogawa L, Prasanna G, Suburo AM (2005) Endothelin-1 and endothelin receptors in light-induced retinal degeneration. Exp Eye Res 81: 265–275 [PubMed]
57. Imai Y, Soda M, Inoue H, Hattori N, Mizuno Y, et al. (2001) An unfolded putative transmembrane polypeptide, which can lead to endoplasmic reticulum stress, is a substrate of Parkin. Cell 105: 891–902 [PubMed]
58. Lepple-Wienhues A, Becker M, Stahl F, Berweck S, Hensen J, et al. (1992) Endothelin-like immunoreactivity in the aqueous humour and in conditioned medium from cultured ciliary epithelial cells. Curr Eye Res 11: 1041–1046 [PubMed]
59. Cellini M, Possati GL, Profazio V, Sbrocca M, Caramazza N, et al. (1997) Color Doppler imaging and plasma levels of endothelin-1 in low-tension glaucoma. Acta Ophthalmol Scand Suppl: 11–13 [PubMed]
60. Sugiyama T, Moriya S, Oku H, Azuma I (1995) Association of endothelin-1 with normal tension glaucoma: clinical and fundamental studies. Surv Ophthalmol 39 Suppl 1: S49–56 [PubMed]
61. Koliakos GG, Konstas AG, Schlotzer-Schrehardt U, Hollo G, Mitova D, et al. (2004) Endothelin-1 concentration is increased in the aqueous humour of patients with exfoliation syndrome. Br J Ophthalmol 88: 523–527 [PMC free article] [PubMed]
62. Tao W, Prasanna G, Dimitrijevich S, Yorio T (1998) Endothelin receptor A is expressed and mediates the [Ca2+]i mobilization of cells in human ciliary smooth muscle, ciliary nonpigmented epithelium, and trabecular meshwork. Curr Eye Res 17: 31–38 [PubMed]
63. Drager UC, Olsen JF (1981) Ganglion cell distribution in the retina of the mouse. Invest Ophthalmol Vis Sci 20: 285–293 [PubMed]
64. Perry VH (1981) Evidence for an amacrine cell system in the ganglion cell layer of the rat retina. Neuroscience 6: 931–944 [PubMed]
65. Jeon CJ, Strettoi E, Masland RH (1998) The major cell populations of the mouse retina. J Neurosci 18: 8936–8946 [PubMed]
66. Rodieck RW (1973) The vertebrate retina; principles of structure and function. San Francisco,: Freeman. x, 1044 p.
67. Fukuroda T, Fujikawa T, Ozaki S, Ishikawa K, Yano M, et al. (1994) Clearance of circulating endothelin-1 by ETB receptors in rats. Biochem Biophys Res Commun 199: 1461–1465 [PubMed]
68. Dupuis J, Goresky CA, Fournier A (1996) Pulmonary clearance of circulating endothelin-1 in dogs in vivo: exclusive role of ETB receptors. J Appl Physiol 81: 1510–1515 [PubMed]
69. Berkelaar M, Clarke DB, Wang YC, Bray GM, Aguayo AJ (1994) Axotomy results in delayed death and apoptosis of retinal ganglion cells in adult rats. J Neurosci 14: 4368–4374 [PubMed]
70. Garcia-Valenzuela E, Shareef S, Walsh J, Sharma SC (1995) Programmed cell death of retinal ganglion cells during experimental glaucoma. Exp Eye Res 61: 33–44 [PubMed]
71. Kermer P, Ankerhold R, Klocker N, Krajewski S, Reed JC, et al. (2000) Caspase-9: involvement in secondary death of axotomized rat retinal ganglion cells in vivo. Brain Res Mol Brain Res 85: 144–150 [PubMed]
72. Watanabe M, Fukuda Y (2002) Survival and axonal regeneration of retinal ganglion cells in adult cats. Prog Retin Eye Res 21: 529–553 [PubMed]
73. Weishaupt JH, Diem R, Kermer P, Krajewski S, Reed JC, et al. (2003) Contribution of caspase-8 to apoptosis of axotomized rat retinal ganglion cells in vivo. Neurobiol Dis 13: 124–135 [PubMed]
74. Salinas-Navarro M, Mayor-Torroglosa S, Jimenez-Lopez M, Aviles-Trigueros M, Holmes TM, et al. (2009) A computerized analysis of the entire retinal ganglion cell population and its spatial distribution in adult rats. Vision Res 49: 115–126 [PubMed]
75. Howell GR, Macalinao DG, Sousa GL, Walden M, Soto I, et al. (2011) Molecular clustering identifies complement and endothelin induction as early events in a mouse model of glaucoma. J Clin Invest 121: 1429–1444 [PMC free article] [PubMed]
76. Gariepy CE, Williams SC, Richardson JA, Hammer RE, Yanagisawa M (1998) Transgenic expression of the endothelin-B receptor prevents congenital intestinal aganglionosis in a rat model of Hirschsprung disease. J Clin Invest 102: 1092–1101 [PMC free article] [PubMed]
77. Husak PJ, Kuo T, Enquist LW (2000) Pseudorabies virus membrane proteins gI and gE facilitate anterograde spread of infection in projection-specific neurons in the rat. J Virol 74: 10975–10983 [PMC free article] [PubMed]
78. McKinnon SJ, Lehman DM, Tahzib NG, Ransom NL, Reitsamer HA, et al. (2002) Baculoviral IAP repeat-containing-4 protects optic nerve axons in a rat glaucoma model. Mol Ther 5: 780–787 [PubMed]
79. Barres BA, Silverstein BE, Corey DP, Chun LL (1988) Immunological, morphological, and electrophysiological variation among retinal ganglion cells purified by panning. Neuron 1: 791–803 [PubMed]
80. Hollander H, Vaaland JL (1968) A reliable staining method for semi-thin sections in experimental neurfanatomy. Brain Res 10: 120–126 [PubMed]
81. Chauhan BC, Levatte TL, Garnier KL, Tremblay F, Pang IH, et al. (2006) Semiquantitative optic nerve grading scheme for determining axonal loss in experimental optic neuropathy. Invest Ophthalmol Vis Sci 47: 634–640 [PubMed]

Articles from PLoS ONE are provided here courtesy of Public Library of Science