Thank you for visiting nature.com. You are using a browser version with limited support for CSS. To obtain the best experience, we recommend you use a more up to date browser (or turn off compatibility mode in Internet Explorer). In the meantime, to ensure continued support, we are displaying the site without styles and JavaScript.

Abstract

Ischemia-induced hypoxia elicits retinal neovascularization and is a major component of several blinding retinopathies such as retinopathy of prematurity (ROP), diabetic retinopathy (DR) and retinal vein occlusion (RVO). Currently, noninvasive imaging techniques capable of detecting and monitoring retinal hypoxia in living systems do not exist. Such techniques would greatly clarify the role of hypoxia in experimental and human retinal neovascular pathogenesis. In this study, we developed and characterized HYPOX-4, a fluorescence-imaging probe capable of detecting retinal-hypoxia in living animals. HYPOX-4 dependent in vivo and ex vivo imaging of hypoxia was tested in a mouse model of oxygen-induced retinopathy (OIR). Predicted patterns of retinal hypoxia were imaged by HYPOX-4 dependent fluorescence activity in this animal model. In retinal cells and mouse retinal tissue, pimonidazole-adduct immunostaining confirmed the hypoxia selectivity of HYPOX-4. HYPOX-4 had no effect on retinal cell proliferation as indicated by BrdU assay and exhibited no acute toxicity in retinal tissue as indicated by TUNEL assay and electroretinography (ERG) analysis. Therefore, HYPOX-4 could potentially serve as the basis for in vivo fluorescence-based hypoxia-imaging techniques, providing a tool for investigators to understand the pathogenesis of ischemic retinopathies and for physicians to address unmet clinical needs.

Introduction

Retinopathy of prematurity (ROP)1,2, proliferative diabetic retinopathy (PDR)3 and retinal vein occlusion (RVO)4 are blinding conditions with neovascular components that develop from ischemia-induced retinal hypoxia. In ROP, ischemia arises from attenuated physiologic blood vessel development in preterm infants receiving supplemental oxygen to compensate for under-developed lung function5,6. When the oxygen therapy is discontinued and the infant is placed in normoxia, the peripheral retina is avascular (ischemia) and becomes hypoxic7. Hyperglycemia and hyperlipidemia are causally linked to capillary dropout and vasoregression in the diabetic retina, leading to focal avascularity (ischemia) and Incipient retinal hypoxia that triggers the onset of PDR. Although the exact etiology of branch RVO is unknown, arteriolar compression at an arteriovenous crossing may lead to the formation of an occlusive thrombus in the affected vein, reducing blood flow (ischemia) and presumably initiating the development of retinal hypoxia8. Retinal hypoxia activates the transcription of hypoxia-regulated pro-angiogenic growth factors/cytokines such as vascular endothelial cell growth factors (VEGF)9 and angiopoietin-like protein-4 (ANGPTL4)10. These factors elicit a neovascular response that manifests in the formation of preretinal neovascular structures that enhance morbidity, often leading to blindness in individuals afflicted with ROP, PDR and RVO. Based on these forgoing considerations, the ability to detect, quantify, track and image retinal hypoxia becomes of paramount importance, as it would allow a better understanding of the pathophysiology of ischemic retinopathies. Furthermore, early detection of hypoxia before the onset of any overt neural or vascular anomalies, could perhaps aid the physician to assess whether prophylactic therapy is indicated. Finally, hypoxia imaging and quantification would be useful in terms of gauging the efficacy of therapy on established disease.

Several analytical platforms have been applied to measuring retinal oxygen pressure (pO2) levels including, but not limited to, the use of oxygen sensitive electrodes11, nuclear magnetic resonance (NMR)12, retinal oximetry13, oxygen-dependent molecular phosphorescence quenching14, doppler optical coherence tomography (D-OCT)15, visible-light optical coherence tomography (vis-OCT)16 and immunohistochemical analysis17. Oxygen electrodes permit the acquisition of reliable data but are invasive and are extremely difficult to use in rodents due to their smaller globes. NMR is minimally invasive, however it is not a direct measure of oxygen pressure and the resolution is appreciably less than optical methods18,19,20. Retinal oximetry and doppler OCT are methods that rely on the differences in the spectral characteristics of oxyhemoglobin and hemoglobin in the intravascular compartment and their relative abundance in arteries compared to veins. These measurements may be performed in living systems, however, they are indirect and mathematical modeling is required to estimate the perivascular oxygen pressure. Phosphorescent quenching relies on intravascular oxygen levels providing only limited assessment of the oxygen pressure in the retinal tissue. Pimonidazole-mediated immunohistochemistry is a common method used to determine retinal hypoxia, but the technique is limited by its exclusively ex vivo method of examination21,22. Though a number of methods have been reported in the literature to visualize tumor hypoxia using positron emission tomography, none have been applied to the detection of retinal hypoxia. Furthermore, they carry the risks associated with use of short-lived isotopes. For these and other reasons, the techniques discussed above are not optimal for measuring retinal hypoxia in living animals in real time.

Previously, we described the development of HYPOX-1, HYPOX-2 and HYPOX-3 as sensitive fluorophore-labeled imaging probes to detect hypoxia23,24. These fluorescent probes are reduced by nitroreductases or azoreductases, facilitating their retention within hypoxic cells of the retina, allowing ex vivo hypoxia detection25. However, their application to in vivo imaging was limited due to poor pharmacokinetic parameters. To achieve the goal of in vivo imaging, we continued our efforts to synthesize and characterize a probe having the correct pharmacokinetic properties to allow enhanced diffusion into capillary-free retinal tissue. To address these needs, we synthesized HYPOX-4 and tested its ability to discriminate between normoxia and hypoxia in vivo, by hypoxia-induced fluorescence enhancement. We tested HYPOX-4 in mouse OIR, a preclinical model of ischemia-induced retinopathy in which retinal hypoxia is a critical pathologic component. Herein we report the results.

Materials and MethodsReagents, equipment and cells

Low glucose DMEM, DMEM/F12, Fetal Bovine Serum (FBS), GlutaMAX, Gentamicin/Amphotericin B and Penicillin-Streptomycin were obtained from GIBCO; Grand Island, NY. The human retinal pigment epithelial cell line, ARPE-19 was purchased from ATCC; Manassas, VA. The human M眉ller cell line (MIO-M1) was kindly provided by Dr. G. A. Limb (Moorfields Institute of Ophthalmology, London, UK)26. The rat retinal neuronal cell line R28 was purchased from KeraFast; Boston, MA. A humidified cell culture chamber with a ProOx 110 oxygen control device was obtained from BioSpherix Inc.; Parish, NY. A Hypoxyprobe immunodetection kit (anti-pimonidazole-adduct antibody) was purchased from Hypoxyprobe Inc.; Burlington, MA. The secondary anti-rabbit IgG conjugated to Alexa Fluor庐 647 (AF647), Prolong Gold mounting media with DAPI and Alexa Fluor庐 488- or 647-conjugated isolectin B4 were purchased from Life Technologies; Grand Island, NY.

Mice

C57BL/6J timed-pregnant dams were purchased from Charles River Laboratories; Chicago, Illinois. All animal procedures used in this study were approved by the Vanderbilt University Institutional Animal Care and Use Committee and were performed in accordance with the ARVO Statement for the Use of Animals in Ophthalmic and Vision Research.

Imaging of retinal hypoxia in mouse OIR

In order to produce OIR, mouse pups and their dams were placed in 75% oxygen from P7 to P1227. On P12, litters were removed to room air and after two hours, HYPOX-4 (60鈥塵g/kg in PBS) was administered to mouse pups by intraperitoneal injection. Twenty-four hours post-injection, in vivo HYPOX-4 dependent fluorescence imaging was performed. Briefly, mice were anesthetized with ketamine/xylazine, eyes were dilated with 1% tropicamide and placed on a warm platform; fluorescent and bright field fundus images were acquired using the Micron IV retinal-imaging system (Phoenix Research Laboratories; Pleasanton, CA). Then, ex vivo imaging of HYPOX-4 dependent fluorescence was performed. The mice were sacrificed, enucleated and the globes were fixed in 10% neutral buffered formalin (NBF). Retinas were dissected and stained directly with Alexa Fluor庐 647-conjugated isolectin B4, then flat-mounted on a microscope slide with Prolong Gold mounting medium (Life Technologies, Grand Island, NY). Images were captured using an epifluorescence Nikon Eclipse Ti-E inverted microscope (Melville, NY).

Some mice received intraperitoneal injections of pimonidazole hydrochloride at a concentration of 60鈥塵g/kg body weight two hours after removal to room air; they were sacrificed one hour later and enucleated. The globes were fixed in 10% NBF for two hours; retinas were dissected and washed with tris-buffered saline (TBS); then they were blocked/permeabilized in 10% donkey serum with 1% Triton X-100 and 0.05% Tween 20 in TBS for 6鈥塰ours and stained with rabbit antibody against pimonidazole-adducts followed by the secondary anti-rabbit IgG conjugated to Alexa Fluor庐 647- and Alexa Fluor庐 488-conjugated isolectin B4. The retinas were mounted on microscope slides with Prolong Gold mounting medium. Images were captured using an epifluorescence Nikon Eclipse Ti-E inverted microscope (Melville, NY).

Retinal cell culture

ARPE-19 cells were cultured in DMEM/F12 supplemented with 10% FBS, 1X GlutaMAX and 1X Gentamicin/Amphotericin B. MIO-M1 and R28 cells were cultured in low glucose DMEM supplemented with 10% FBS, 1X GlutaMAX and 1X Penicillin-Streptomycin. Cells were maintained in a humidified environment with 5% CO2 at 37鈥壜癈 unless otherwise noted. The cells were cultured in 96 well plates or 8 well chamber slides and treated with HYPOX-4 concentrations ranging from 10 to 100鈥壩糓 in complete medium containing supplemental nutrients. To establish a hypoxic environment, a calibrated proOx sensor (BioSpherix Inc.; Parish, NY) was used to maintain lower oxygen pressures. The oxygen level was monitored using the TraceableTM Dissolved Oxygen Meter Pen (Fisher Scientific; Pittsburgh, PA). To confirm induction of hypoxia, cells were cultured on chamber slides and treated with 100鈥壩糓 pimonidazole hydrochloride diluted in complete medium, then subjected to hypoxia or normoxia for 4鈥塰ours and immunostained for pimonidazole-adducts according to manufacturer鈥檚 protocol.

In vitro hypoxia-induced, HYPOX-4 dependent fluorescence assay

ARPE-19 and MIO-M1 cells were seeded at 20,000 and R28 at 15,000 cells per well, respectively, in a clear bottom 96-well black plate. When cells were 80% confluent, they were treated with 100鈥壩糓 HYPOX-4 unless otherwise specified, in complete medium and incubated in normoxia or hypoxia for 4鈥塰ours. The cells were washed with pre-warmed Hank鈥檚 Buffered Salt Solution (HBSS). Fluorescence intensity was measured (Absorbance: 490鈥塶m, Emission: 520鈥塶m) using a microplate reader (Biotek; Winooski, VT).

In vitro imaging of retinal cells using HYPOX-4

R28 cells were seeded at a density of 45,000 cells per well in 4-well chamber slides. When cells were 90% confluent, cells were treated with HYPOX-4 in complete medium, or with pimonidazole hydrochloride diluted in complete medium. The cells were cultured in normoxia or hypoxia for 4鈥塰ours. Cells were washed 3 times with HBSS, fixed with 10% NBF for 10鈥塵inutes at room temperature, washed 3 times with TBS and mounted with Prolong Gold with DAPI mounting media. Pimonidazole-adducts were immunostained according to manufacturer鈥檚 protocol. HYPOX-4 dependent fluorescence images were captured using the epifluorescence microscope.

Electroretinography (ERG) measurements

ERG measurements were performed according to previously published methods28,29. Briefly, ERG analysis was performed on mice injected with HYPOX-4 (100鈥塵g/kg) at one week post-injection. Animals were dark adapted overnight, anesthetized with ketamine/xylazine, dilated with 1% tropicamide and placed on a warm platform within the Ganzfeld dome of a Diagnosys LLC Espion Electrophysiology system (Lowell, MA, USA). Mice were exposed to flashes of light ranging from 鈭? to 2 log cd.s/m2 and the amplitudes of a-wave and b-wave were measured from baseline to peak. The amplitude of the a-wave and b-wave were plotted as a function of luminance.

TUNEL assay

TUNEL assays were performed using Click-iT in situ apoptosis detection kit (Life Technology, USA). Adult C57BL/6J mice were treated with HYPOX-4 (100鈥塵g/kg); they were sacrificed 24鈥塰our later and enucleated. The eyes were fresh frozen in 30% sucrose and embedded in TissueTec OCT for cryosectioning (7鈥壩糾 sections). The retinal transverse sections were then stained for fragmented DNA by incorporating alkyne-modified EdUTP nucleotide followed by detection with Alexa Fluor庐 647 azide in apoptotic cells. Retinal transverse sections from C57BL/6J mice that did not receive HYPOX-4 were treated with DNase I and stained as a positive control. Counts of TUNEL鈥?鈥塶uclei were performed by counting total number of stained nuclei across 400鈥壩糾 sections of each individual sample.

Cell proliferation assay

Retinal cell-lines were treated with HYPOX-4 (100鈥壩糓) and proliferation was measured using the bromodeoxyUridine (BrdU) incorporation assay according to the manufacturers protocol. Briefly, retinal cells were seeded in a 96-well plate, cultured for twenty four hours. Then, cells were treated with HYPOX-4 or vehicle controls diluted in complete media and allowed to incubate for 24鈥塰. Four hours prior to the end of the incubation, BrdU was added at a concentration of 10鈥壩糓 and incorporation of BrdU was quantified by ELISA with the BrdU cell proliferation ELISA kit (Exalpha Biologicals; Shirley, MA) according to manufacturer鈥檚 protocol.

Statistics

Data are presented as mean鈥壜扁€塖D. Student鈥檚 t tests were performed to compare 2 samples and, for comparison of more than 2 samples, one-way ANOVA was performed using Prism 6 (Graph- Pad, San Diego, CA). p鈥夆墹鈥?.05 was considered as statistically significant.

Synthesis of HYPOX-4

The synthesis and related characterization data for HYPOX-4 is supplied in the supplementary information (SI).

ResultsIn vitro hypoxia-induced HYPOX-4 fluorescence activity

Cultures of rat retinal neuronal cells (R28) were treated with 100鈥壩糓 HYPOX-4 and exposed to variable oxygen concentrations ranging from 0.1% to 20.9% for 4鈥塰ours. HYPOX-4 dependent fluorescence was maximal at 0.1% oxygen (Fig. 1A). Next, using R28 cells (Fig. 1B), retinal pigment epithelial cells (ARPE-19, Fig. 1C) and human M眉ller cells (MIO-M1, Fig. 1D), the oxygen concentration was maintained at 0.1% and the HYPOX-4 concentration was varied from 10鈥壩糓 to 100鈥壩糓. HYPOX-4 dependent fluorersecence was observed with highest signal to noise ratios at the100鈥壩糓 dose, for all cell types. Additionally, we also observed increased fluorescence in the normoxic cells at the highest concentration (100鈥壩糓) that we applied. This may be due to baseline azoreductase activity causing increased retention of HYPOX-4 that becomes more significant at the highest concentration. Finally, we performed in vitro cellular imaging using R28 cells. Hypoxia-specific, HYPOX-4 dependent fluorescence activity facilitated hypoxia imaging in this cell-line, as shown in Fig. 1E,F. The punctate bright green fluorescence was consistently obseved in these R28 cultures using pimonidazole and several other hypoxia sensing probes and also the R28 cell line is known to be a heterogeneous cell population23. Therefore, this fluorescence may represent cell-associated hypoxic signal. Minimal HYPOX-4 dependent fluorescence was observed in normoxic cells (Fig. 1G,H). Hypoxia was confirmed in these cell lines by immunostaining pimonidazole-adducts (Figure S5)24. All in vitro experiments were replicated a minimum of three times. Where appropriate, results were statistically evaluated by ANOVA.

Figure 1

Sensitivity and hypoxia-specificity of HYPOX-4 in retinal cells.

(A) R28 cells were treated with HYPOX-4 (100鈥壩糓) and variable oxygen concentrations. HYPOX-4 dependent fluorescence increased with decreasing oxygen concentration. (B) R28, (C) ARPE19 and (D) MIO-M1 cells were treated with concentrations of HYPOX-4 ranging from 10 to 100鈥壩糓 and 0.1% oxygen concentration; a HYPOX-4 dose-dependent fluorescence was observed in all of these cell types. (E,F) R28 cells were treated with HYPOX-4 (100鈥壩糓) and 0.1% oxygen for 4鈥塰ours. Hypoxia-specific fluorescence cell imaging was achieved. (G,H) Minimal fluorescence was observed in normoxic cells (n鈥?鈥?, *p鈥?lt;鈥?.05).

Full size imageIn vivo imaging of retinal hypoxia in the mouse model of oxygen induced retinopathy (OIR)

In vivo imaging of retinal hypoxia was performed in OIR mice21. HYPOX-4 was administered by intraperitoneal injection 2鈥塰ours after mice were returned from oxygen exposure chambers to room air (P12); age-matched room air (RA) control pups were similarly treated. In vivo fluorescence imaging was performed 24鈥塰ours post HYPOX-4 injection. HYPOX-4 dependent fluorescence was observed and it was localized to the central avascular retina where the capillary bed was attenuated (Fig. 2). In vivo and ex vivo HYPOX-4 dependent fluorescence was undetectable in age matched RA (P13) control pups. Retinal hypoxia in OIR pups was confirmed by ex vivo pimonidazole-adduct immunostaining. The en face images were highly similar to those obtained by in vivo HYPOX-4 dependent fluorescence (Fig. 2I), both overlapping with regions of retinal avascularity. These results indicate that HYPOX-4 may be used to reliably assess and image retinal hypoxia in a living system in real time.

Figure 2

In vivo imaging of retinal hypoxia in mouse OIR (P13) and age matched room air (RA) pups.

HYPOX-4 was administered systemically to OIR mouse pups 2鈥塰ours after return to room air on P12, as well as to age-matched room air pups. In vivo imaging was performed 24鈥塰ours post-injection of HYPOX-4. (A) Bright field image of OIR (P13) retina; (B) An image of the same retina in vivo, hypoxia was clearly detected by HYPOX-4 dependent fluorescence within the central avascular retina (green); (C) Bright field image of age-matched RA pup (P13); (D) HYPOX-4 dependent fluorescence was undetectable in aged-matched RA pups; (E) OIR mouse retina showing ex vivo HYPOX-4 dependent fluorescence in the central avascular retina (green); (F) The same retina counterstained with IB4, highlighting the peripheral vascular retina; (G) E and F merged; (H) RA pups showed minimal ex vivo HYPOX-4 dependent fluorescence; IB4 staining of the retinal vasculature (red) from an RA pup; (I) Hypoxia was confirmed in OIR (P12) pups by immunostaining of pimonidazole-adducts (red); blood vessels were counterstained with IB4 (green).

Full size imageEx vivo HYPOX-4 dependent fluorescence imaging of retinal transverse sections

Ex vivo fluorescence imaging of transverse retinal sections from OIR pups treated with HYPOX-4 was performed. HYPOX-4 dependent fluorescence indicated laterally alternating regions of hypoxia in the inner retina (Fig. 3A). Within a hypoxic region, proceeding from the inner limiting membrane (ILM) in a sclerad direction, hypoxia was observed in the inner plexiform and inner nuclear layers. Hypoxia was not observed sclerad to the inner nuclear layer. The presence of hypoxia in the inner retina was confirmed using pimonidazole-adduct immunostaining in transverse OIR retinal sections (Fig. 3B). The ex vivo patterns of retinal hypoxia obtained confirmed hypoxia in the inner plexiform and inner nuclear layers. The pimonidazole method also detected hypoxia in the retinal ganglion cell layer.

Figure 3

Localization of HYPOX-4 and pimonidazole in transverse retinal sections from OIR mice.

OIR pups (P12) were treated with HYPOX-4 or pimonidazole and the spatial distribution of hypoxia was determined in retinal cross-sections. (A) HYPOX-4 dependent fluorescence activity indicated alternating regions of hypoxia in the inner retina overlapping with retinal avascularity (green); hypoxia was visualized in the inner plexiform and inner nuclear layers. Presumably, oxygen diffusion out of the major vessel indicated by the white arrow, inhibits increased azo/nitroreductase activities and consequently the retention of HYPOX-4. (B) Pimonidazole-adduct immunostaining confirmed retinal hypoxia in the inner plexiform and inner nuclear layers; additionally, this method detected hypoxia in the ganglion cell layer (red). (A,B) retinal nuclei were stained with DAPI (blue). Abbreviations: GCL鈥?鈥塯anglion cell layer, IPL鈥?鈥塱nner plexiform layer, INL鈥?鈥塱nner nuclear layer, OPL鈥?鈥塷uter plexiform layer, ONL鈥?鈥塷uter nuclear layer.

Full size imageToxicity of HYPOX-4

In vivo toxicity was assessed by electroretinography (ERG) measurements in retinas from RA mice. HYPOX-4 probe (100鈥塵g/kg) was injected systemically and ERG measurements were recorded in dark-adapted mice seven days post-administration. No significant changes in mean a-wave and b-wave amplitudes at various flash intensities were observed as compared to vehicle-treated mice (Fig. 4A,B). Ex vivo analysis of transverse retinal sections from RA mice treated with HYPOX-4 was performed to detect retinal cell apoptosis using the TUNEL assay. No apoptosis was observed, indicating no acute toxicity as compared to the positive control retinal tissues (Fig. 4C鈥揌). Cell proliferation assays were performed in R28 and MIO-M1 retinal cells treated with variable concentration of HYPOX-4 ranging from 0鈥?00鈥壩糓; BrdU incorporation was analyzed. HYPOX-4 had no effect on cell proliferation (Fig. 4I,J). The ERG experiments were replicated three times. The results were statistically evaluated by ANOVA for mean a-wave and b-wave amplitudes at various flash intensities in different treatments groups. The cell proliferation assays were replicated three times and were evaluated by Student鈥檚 t-test for statistical significance.

Figure 4

Effect of HYPOX-4 on retinal physiology was assayed in RA-raised mice via electroretinography (ERG) analysis.

(A,B) ERG measurements of dark-adapted mice 7 days post systemic administration of HYPOX-4 revealed no significant changes in mean a-wave and b-wave amplitudes at various flash intensities compared to vehicle (PBS) and sodium fluorescein (control) groups. The TUNEL assay was performed in retinal transverse sections to assess retinal apoptosis and taken as a measure of retinal toxicity. RA mice were treated with 100鈥壩糓 HYPOX-4 or DNase 1; HYPOX-4 showed no cellular apoptosis. (C,F) DAPI staining of nuclei; (D) DNase 1-treated retinal transverse sections serving as a positive control, fragmented DNA was clearly visible; (G) HYPOX-4 treated retinal transverse sections showed no cellular apoptosis; (E) C and D merged; (H) F and G merged. (I,J) In vitro cellular proliferation was assessed by the BrdU assay using HYPOX-4 treated R28 and MIO-M1 cells. No effect on cellular proliferation was observed.

Full size imageDiscussion

The synthetic strategy of HYPOX-4 was predicated on the need for a molecule with hypoxia-sensitive functionality, superior hypoxia-induced fluorescence and pharmacokinetic properties that would allow optimal tissue diffusion and bioavailablity, all required for in vivo imaging. Oregon Green dye has several advantages for its application to biological systems. It has: a high extinction coefficient, high fluorescence quantum yield, pH insensitivity in the physiological range, high photostability and good tissue penetration. The 2-nitroimidazole moiety was incorporated into the structure of HYPOX-4 because it is reduced by nitroreductase, an enzyme activity that is increased in tissue hypoxia, allowing 2-nitroimidazole to yield hypoxia-sensitive functionality. The solubility of HYPOX-4 was compared directly with the clinically relevant pimonidazole hydrochloride, using the octanol-water partition coefficient measurement method. Similar to pimonidazole hydrochloride, HYPOX-4 is highly soluble in aqueous medium in the free base form (Figure S3, Table SI 1). HYPOX-4 also possesses high photostability at room temperature in solution for at least 20鈥塰ours as determined by kinetic fluorescence studies (Figure S6).

We tested the hypoxia-dependent fluorescence of HYPOX-4 in ARPE-19, MIO-M1 and R28 cells (Fig. 1). We found that HYPOX-4 was efficiently internalized by these cells and an enhanced fluorescence reporter activity was observed in hypoxic cells at 鈮?% (pO2鈥夆墹鈥?8鈥塵mHg) as compared to normoxic controls. We confirmed that hypoxia was achieved in these retinal cell lines by pimonidazole-adduct immunostaining (Figure S5)24. These in vitro studies provided evidence for the feasibility of HYPOX-4 to report the hypoxic condition in a living system, warranting the extension of these studies to the in vivo setting using a rodent model of ischemic retinopathy. HYPOX-4 was tested in cell proliferation assays and had no effect on cell proliferation (Fig. 4I,J).

We performed in vivo experiments to determine whether hypoxia-dependent HYPOX-4 fluorescence could be observed in living animals predisposed to ischemic retinopathy. We tested HYPOX-4 in an established mouse model of oxygen-induced retinopathy (OIR)27. In this model, OIR mice are exposed to 75% oxygen for five days from P7 to P12, causing vaso-attenuation, resulting in a central avascular retina. On P12, the mice are placed in normoxia and ex vivo pimonidazole-adduct immunostaining experiments indicate the central avascular retina becomes hypoxic within a few hours21,30,31. We systemically administered HYPOX-4 to OIR mice 2鈥塰ours after return to room air (P12) and to age-matched normoxic controls. After 24鈥塰ours post-HYPOX-4 administration, in vivo imaging clearly demonstrated a HYPOX-4 dependent fluorescence within the central avascular retina and this fluorescence was absent in adjacent perfused retinal regions. This observation clearly indicates hypoxia in the central avascular retina (Fig. 2). Ex vivo evaluation of HYPOX-4 fluorescence from the same retinas was in close agreement with the in vivo findings and IB4 counterstaining confirmed localization of hypoxia to the central capillary-free regions of the retina. These results agree with similar findings we obtained using the ex vivo pimonidazole-adduct immunostaining technique. In vivo and ex vivo HYPOX-4 fluorescence was undetectable in age-matched RA controls after twenty-four hours of administration. In OIR retinas, the fluorescence signal was barely detectable after seventy-two hours.

In transverse retinal sections from OIR mice, HYPOX-4 dependent fluorescence indicated hypoxic cells in the inner nuclear layer with processes extending to the inner plexiform layer (Fig. 3A, Figure S4)21. Hypoxia was also assessed by pimonidazole-adduct immunostaining. This method confirmed hypoxia in the inner nuclear and plexiform layers (Fig. 3B); however, it was also detected in the retinal ganglion cell layer, creating a discrepancy between the results obtained by the two techniques. These results indicate that HYPOX-4 might discriminate between different levels of hypoxia in the inner nuclear layer and the retinal ganglion cell layer. In C57BL/6 OIR mice (the strain used in this study) it is plausible that there is lower oxygen pressure at the inner nuclear and plexiform layers compared to the retinal ganglion cell layer on day P12 through P13 (the first twenty four hours post oxygen exposure), corresponding to the times we assessed hypoxia, for the following reasons. The superficial vascular plexus is almost fully developed at the time oxygen treatment is initiated on P732. Alternatively, the deep and intermediate vascular plexi have just begun to form and exposure to hyperoxia suppresses their continued development. Vasoobliteration of the superficial plexi is maximal in the central retina two days post initiation of hyperoxia and there is evidence that revascularization (superficial plexi) begins shortly thereafter31. Given these considerations, it is most likely that ganglion cells adjacent to any residual or regenerated superficial vascular plexus, experience higher oxygen pressures than the inner nuclear and plexiform layers in OIR mice at the time we assessed hypoxia. Furthermore, even in normal adult mice and rats with a fully developed retinal vasculature, the oxygen pressures are lower at the inner nuclear layer compared to the ganglion cell layer33,34. Additionally, it is unlikely that the pO2 at the RGC layer is appreciably affected by an oxygen source other than the retinal vasculature. Measurements of oxygen levels in experimental models and in normal human eyes, suggest that oxygen diffuses out of the retinal arterioles and into the vitreous where it is consumed by the nearby retinal tissues, creating an oxygen gradient that decreases from the posterior to the anterior segment of the eye35. In a kitten OIR model, using O2 microelectrodes to measure retinal pO2, preretinal pO2 levels approached 0鈥塵mHg immediately above the avascular area, indicating that oxygen is not delivered to the RGC layer from a vitreous source in the absence of the retinal vasculature36,37. Taken together, these data suggest that the vitreous is not an independent source of oxygen that provides increased pO2 at the RGC layer.

Therefore, the discrepancies we observed on comparison of HYPOX-4 dependent fluorescence imaging and pimonidazole-adduct immunostaining in transverse retinal sections may be best explained by a lower oxygen pressure detection threshold for HYPOX-4 relative to pimonidazole. This explaination is further supported by our in vitro studies. HYPOX-4 dependent fluorescence was observed at a threshold of pO2鈥夆墹鈥?8鈥塵mHg in retinal cell lines cultured in hypoxia (normoxia; pO2鈥夆増鈥?60鈥塵mHg); whereas pimonidazole detects hypoxia at pO2鈥?lt;鈥?6鈥塵mHg. We also propose that this lower detection limit is advantageous for the detection of oxygen pressures that are functionally significant to neovascular pathogies. For example, experimental evidence indicates that hypoxia induces M眉ller cells and astrocytes to express and secrete increased retinal VEGF levels that promote preretinal neovascularization in experimental ischemic retinopathies. A previous study indicated that hypoxic induction of VEGF, in an immortalized M眉ller cell line was nominally significant at pO2鈥檚鈥夆墹鈥?8鈥塵mHg38. Accordingly, retinal pO2鈥檚 ranging from 76 to 38鈥塵mHg, detectable by pimonidazole but not HYPOX-4, are not likely to be related to disease processes. In fact, it is known that oxgen pressures in the normal adult rodents fall within this range. We did not perfom retinal pO2 measurements in our experimental cohorts, although these data are valuble for determing the actual in vivo pO2 ranges detected by HYPOX-4. These measurements are very difficult in adult rodents and present an even more formidable challenge in P12鈥揚18 mouse pups. However, published measurements in the normal adult mouse indicate a pO2鈥夆増鈥?.0鈥塵mHg at the inner nuclear layer34. Therefore, it is plausible that pO2 in mouse OIR pups is 5.0鈥塵mHg at the inner nuclear layer, given that development of the deep capillary plexus is substantially retarded in this model. In our in vitro work, we observed maximum HYPOX-4-dependent fluorescence at 1鈥塵mHg. Hence, it is reasonable to expect that the ranges of oxygen pressures observed in vitro and in vivo by HYPOX-4-dependent fluorescence overlap.

Electroretinography (ERG) measurements in dark-adapted RA mice seven days post systemic administration of HYPOX-4 revealed no significant changes in mean a-wave and b-wave amplitudes compared to vehicle indicating no acute effect of HYPOX-4 on retinal physiology (Fig. 4A,B). Ex vivo analysis of the retinal transverse sections from RA mice treated with HYPOX-4, were also examined using the TUNEL assay. No significant toxicity related to apoptosis was observed as compared to the positive control tissues (Fig. 4C鈥揌). Furthermore, HYPOX-4 had no effect on in vitro cell-proliferation indicating that it would not affect retinal mitogenesis.

In summary, we have developed a facile route for the synthesis of HYPOX-4, a hypoxia-sensitive imaging agent, by conjugating 2-nitroimidazole to the fluorescent dye, Oregon green. HYPOX-4 is a novel probe that is not acutely toxic to retinal tissues and demonstrates pharmacokinetic properties required for efficient systemic delivery and bioavailabilty within the retina. Using HYPOX-4, we were able to detect retinal hypoxia in vivo in mouse model of OIR. To our knowledge, this is the first report of real time hypoxia imaging in living animals by a fluorescence-based method in the retina. HYPOX-4 hypoxia-induced retinal imaging is non-invasive and it promises to be an excellent tool for diagnosis and monitoring retinal hypoxia in preclinical disease models and patients.

Additional Information

How to cite this article: Uddin, M. I. et al. In Vivo Imaging of Retinal Hypoxia in a Model of Oxygen-Induced Retinopathy. Sci. Rep. 6, 31011; doi: 10.1038/srep31011 (2016).

References

Gariano, R. F. Gardner, T. W. Retinal angiogenesis in development and disease. Nature 438, 960鈥?66, doi: 10.1038/nature04482 (2005).

CASArticleADSPubMedPubMed Central Google Scholar

Anderson, C. G., Benitz, W. E. Madan, A. Retinopathy of prematurity (ROP) and pulse oximetry: A national survey of recent practices. Pediatr Res 51, 367a鈥?67a (2002).

Google Scholar

Wang, X. Q., Wang, G. B. Wang, Y. Intravitreous Vascular Endothelial Growth Factor and Hypoxia-Inducible Factor 1a in Patients With Proliferative Diabetic Retinopathy. Am J Ophthalmol 148, 883鈥?89, doi: 10.1016/j.ajo.2009.07.007 (2009).

CASArticlePubMedPubMed Central Google Scholar

Rehak, J. Rehak, M. Branch retinal vein occlusion: Pathogenesis, visual prognosis and treatment modalities. Curr Eye Res 33, 111鈥?31, doi: 10.1080/02713680701851902 (2008).

ArticlePubMedPubMed Central Google Scholar

Hartnett, M. E. Penn, J. S. Mechanisms and Management of Retinopathy of Prematurity. New Engl J Med 367, 2515鈥?526, doi: 10.1056/Nejmra1208129 (2012).

CASArticlePubMedPubMed Central Google Scholar

Ashton, N. Cook, C. Direct observation of the effect of oxygen on developing vessels: preliminary report. The British journal of ophthalmology 38, 433鈥?40 (1954).

CASArticlePubMedPubMed Central Google Scholar

Ashton, N. Pathological basis of retrolental fibroplasia. The British journal of ophthalmology 38, 385鈥?96 (1954).

CASArticlePubMedPubMed Central Google Scholar

O鈥橫ahoney, P. R. A., Wong, D. T. Ray, J. G. Retinal vein occlusion and traditional risk factors for atherosclerosis. Arch Ophthalmol-Chic 126, 692鈥?99, doi: 10.1001/archopht.126.5.692 (2008).

Article Google Scholar

Robbins, S. G., Conaway, J. R., Ford, B. L., Roberto, K. A. Penn, J. S. Detection of vascular endothelial growth factor (VEGF) protein in vascular and non-vascular cells of the normal and oxygen-injured rat retina. Growth Factors 14, 229- , doi: 10.3109/08977199709021522 (1997).

CASArticlePubMedPubMed Central Google Scholar

Xin, X. B. et al. Hypoxic retinal Muller cells promote vascular permeability by HIF-1-dependent up-regulation of angiopoietin-like 4. P Natl Acad Sci USA 110, E3425鈥揈3434, doi: 10.1073/pnas.1217091110 (2013).

Article Google Scholar

Linsenmeier, R. A. et al. Retinal hypoxia in long-term diabetic cats. Invest Ophth Vis Sci 39, 1647鈥?657 (1998).

CAS Google Scholar

Berkowitz, B. A. Penn, J. S. Abnormal panretinal response pattern to carbogen inhalation in experimental retinopathy of prematurity. Invest Ophthalmol Vis Sci 39, 840鈥?45 (1998).

CASPubMedPubMed Central Google Scholar

Hardarson, S. H. et al. Automatic retinal oximetry. Invest Ophthalmol Vis Sci 47, 5011鈥?016, doi: 10.1167/iovs.06-0039 (2006).

ArticlePubMedPubMed Central Google Scholar

Shahidi, M., Shakoor, A., Blair, N. P., Mori, M. Shonat, R. D. A method for chorioretinal oxygen tension measurement. Curr Eye Res 31, 357鈥?66, doi: 10.1080/02713680600599446 (2006).

CASArticlePubMedPubMed Central Google Scholar

Dai, C., Liu, X., Zhang, H. F., Puliafito, C. A. Jiao, S. Absolute retinal blood flow measurement with a dual-beam Doppler optical coherence tomography. Invest Ophthalmol Vis Sci 54, 7998鈥?003, doi: 10.1167/iovs.13-12318 (2013).

ArticlePubMedPubMed Central Google Scholar

Soetikno, B. T. et al. Inner retinal oxygen metabolism in the 50/10 oxygen-induced retinopathy model. Scientific reports 5, 16752, doi: 10.1038/srep16752 (2015).

CASArticleADSPubMedPubMed Central Google Scholar

Scott, A. Fruttiger, M. Oxygen-induced retinopathy: a model for vascular pathology in the retina. Eye 24, 416鈥?21, doi: 10.1038/eye.2009.306 (2010).

CASArticlePubMedPubMed Central Google Scholar

Busk, M. et al. PET imaging of tumor hypoxia using 18F-labeled pimonidazole. Acta oncologica 52, 1300鈥?307, doi: 10.3109/0284186X.2013.815797 (2013).

CASArticlePubMedPubMed Central Google Scholar

Kizaka-Kondoh, S. Konse-Nagasawa, H. Significance of nitroimidazole compounds and hypoxia-inducible factor-1 for imaging tumor hypoxia. Cancer science 100, 1366鈥?373, doi: 10.1111/j.1349-7006.2009.01195.x (2009).

CASArticlePubMedPubMed Central Google Scholar

Yang, Y. et al. Magnetic resonance imaging retinal oximetry: a quantitative physiological biomarker for early diabetic retinopathy? Diabetic medicine: a journal of the British Diabetic Association 29, 501鈥?05, doi: 10.1111/j.1464-5491.2011.03440.x (2012).

CASArticle Google Scholar

Mowat, F. M. et al. HIF-1alpha and HIF-2alpha are differentially activated in distinct cell populations in retinal ischaemia. PloS one 5, e11103, doi: 10.1371/journal.pone.0011103 (2010).

CASArticleADSPubMedPubMed Central Google Scholar

Varia, M. A. et al. Pimonidazole: A novel hypoxia marker for complementary study of tumor hypoxia and cell proliferation in cervical carcinoma. Gynecol Oncol 71, 270鈥?77, doi: 10.1006/gyno.1998.5163 (1998).

CASArticlePubMedPubMed Central Google Scholar

Uddin, M. I. et al. Applications of Azo-Based Probes for Imaging Retinal Hypoxia. Acs Med Chem Lett 6, 445鈥?49, doi: 10.1021/ml5005206 (2015).

CASArticlePubMedPubMed Central Google Scholar

Evans, S. M. et al. Molecular Probes for Imaging of Hypoxia in the Retina. Bioconjugate Chem 25, 2030鈥?037, doi: 10.1021/bc500400z (2014).

CASArticle Google Scholar

Ross, D., Beall, H. D., Siegel, D., Traver, R. D. Gustafson, D. L. Enzymology of bioreductive drug activation. The British journal of cancer. Supplement 27, S1鈥揝8 (1996).

CASPubMedPubMed Central Google Scholar

Limb, G. A., Salt, T. E., Munro, P. M., Moss, S. E. Khaw, P. T. In vitro characterization of a spontaneously immortalized human Muller cell line (MIO-M1). Invest Ophthalmol Vis Sci 43, 864鈥?69 (2002).

PubMedPubMed Central Google Scholar

Smith, L. E. et al. Oxygen-induced retinopathy in the mouse. Invest Ophthalmol Vis Sci 35, 101鈥?11 (1994).

CASPubMedPubMed Central Google Scholar

Domenici, L., Berardi, N., Carmignoto, G., Vantini, G. Maffei, L. Nerve growth factor prevents the amblyopic effects of monocular deprivation. Proc Natl Acad Sci USA 88, 8811鈥?815 (1991).

CASArticleADSPubMedPubMed Central Google Scholar

Rex, T. S. et al. Systemic but not intraocular Epo gene transfer protects the retina from light-and genetic-induced degeneration. Molecular therapy: the journal of the American Society of Gene Therapy 10, 855鈥?61, doi: 10.1016/j.ymthe.2004.07.027 (2004).

CASArticle Google Scholar

Connor, K. M. et al. Quantification of oxygen-induced retinopathy in the mouse: a model of vessel loss, vessel regrowth and pathological angiogenesis. Nature protocols 4, 1565鈥?573, doi: 10.1038/nprot.2009.187 (2009).

CASArticlePubMedPubMed Central Google Scholar

Stahl, A. et al. The mouse retina as an angiogenesis model. Invest Ophthalmol Vis Sci 51, 2813鈥?826, doi: 10.1167/iovs.10-5176 (2010).

ArticlePubMedPubMed Central Google Scholar

Penn, J. S. et al. Vascular endothelial growth factor in eye disease. Prog Retin Eye Res 27, 331鈥?71, doi: 10.1016/j.preteyeres.2008.05.001 (2008).

CASArticlePubMedPubMed Central Google Scholar

Lau, J. C. Linsenmeier, R. A. Oxygen consumption and distribution in the Long-Evans rat retina. Exp Eye Res 102, 50鈥?8, doi: 10.1016/j.exer.2012.07.004 (2012).

CASArticlePubMedPubMed Central Google Scholar

Yu, D. Y. Cringle, S. J. Oxygen distribution in the mouse retina. Invest Ophthalmol Vis Sci 47, 1109鈥?112, doi: 10.1167/iovs.05-1118 (2006).

ArticlePubMedPubMed Central Google Scholar

Beebe, D. C., Shui, Y. B., Siegfried, C. J., Holekamp, N. M. Bai, F. Preserve the (intraocular) environment: the importance of maintaining normal oxygen gradients in the eye. Japanese Journal of Ophthalmology 58, 225鈥?31, doi: 10.1007/s10384-014-0318-4 (2014).

CASArticlePubMedPubMed Central Google Scholar

Wangsa-Wirawan, N. D. Linsenmeier, R. A. Retinal oxygen: fundamental and clinical aspects. Arch Ophthalmol 121, 547鈥?57, doi: 10.1001/archopht.121.4.547 (2003).

ArticlePubMedPubMed Central Google Scholar

Ernest, J. T. Goldstick, T. K. Retinal oxygen tension and oxygen reactivity in retinopathy of prematurity in kittens. Invest Ophthalmol Vis Sci 25, 1129鈥?134 (1984).

CASPubMedPubMed Central Google Scholar

Eichler, W., Yafai, Y., Keller, T., Wiedemann, P. Reichenbach, A. PEDF derived from glial Muller cells: a possible regulator of retinal angiogenesis. Exp Cell Res 299, 68鈥?8, doi: 10.1016/j.yexcr.2004.05.020 (2004).

CASArticlePubMedPubMed Central Google Scholar

Download references

Acknowledgements

This work was supported by National Institutes of Health Grants R01EY23397, R01EY07533 and R01EY23639 (to JSP), CA128323-4,-5 and CA182850-01A1 (to MJU), MMPC MICROMouse U24DK076169 (to AJ), Vanderbilt Diabetes Research and Training Center Core grant (P30 DK020593-34-39), a Grants from the Carl Marshall Reeves Mildred Almen Reeves Foundation, Inc. (to JSP) and an Unrestricted Grant from Research to Prevent Blindness, Inc. Spectroscopic analysis was conducted in the Small Molecule NMR Facility and Mass Spectrometry Research Center at the Vanderbilt Institute of Chemical Biology.

Author informationAffiliationsDepartment of Ophthalmology and Visual Sciences, Vanderbilt University School of Medicine, Nashville, TN, USAMd. Imam Uddin,聽Stephanie M. Evans,聽Jason R. Craft,聽Gary W. McCollum,聽Rong Yang聽 聽John S. PennDepartment of Molecular Physiology and Biophysics, Vanderbilt University School of Medicine, Nashville, TN, USAMegan E. Capozzi聽 聽John S. PennDepartments of Biochemistry, A. B. Hancock, Jr., Memorial Laboratory for Cancer Research, Chemistry and Pharmacology, Vanderbilt Institute of Chemical Biology, Center for Molecular Toxicology and Vanderbilt-Ingram Cancer Center, Vanderbilt University School of Medicine, Nashville, TN, USALawrence J. Marnett聽 聽Md. Jashim UddinPharma Research and Early Development, Roche Innovation Center Basel, F. Hoffmann-La Roche, Ltd., Basel, SwitzerlandAshwath JayagopalAuthorsMd. Imam UddinView author publicationsYou can also search for this author in PubMed Google Scholar Stephanie M. EvansView author publicationsYou can also search for this author in PubMed Google Scholar Jason R. CraftView author publicationsYou can also search for this author in PubMed Google Scholar Megan E. CapozziView author publicationsYou can also search for this author in PubMed Google Scholar Gary W. McCollumView author publicationsYou can also search for this author in PubMed Google Scholar Rong YangView author publicationsYou can also search for this author in PubMed Google Scholar Lawrence J. MarnettView author publicationsYou can also search for this author in PubMed Google Scholar Md. Jashim UddinView author publicationsYou can also search for this author in PubMed Google Scholar Ashwath JayagopalView author publicationsYou can also search for this author in PubMed Google Scholar John S. PennView author publicationsYou can also search for this author in PubMed Google Scholar Contributions

M.I.U. designed and supervised the project, performed the imaging studies, analyzed the data and wrote the manuscript; S.M.E. performed the cell culture and in vitro assays; J.R.C. performed the animal husbandry and ex vivo assays; M.E.C. performed the induction of retinopathy in OIR mice; G.W.M. helped revised the manuscript, R.Y. performed dissection of the retina, L.J.M., M.J.U., A.J. and J.S.P. supervised the project; All authors reviewed the manuscript.

Ethics declarations Competing interests

The authors declare no competing financial interests.

Electronic supplementary material Supplementary InformationRights and permissions

This work is licensed under a Creative Commons Attribution 4.0 International License. The images or other third party material in this article are included in the article鈥檚 Creative Commons license, unless indicated otherwise in the credit line; if the material is not included under the Creative Commons license, users will need to obtain permission from the license holder to reproduce the material. To view a copy of this license, visit http://creativecommons.org/licenses/by/4.0/

Reprints and Permissions

About this articleCite this article

Uddin, M., Evans, S., Craft, J. et al. In Vivo Imaging of Retinal Hypoxia in a Model of Oxygen-Induced Retinopathy. Sci Rep 6, 31011 (2016). https://doi.org/10.1038/srep31011

Download citation

Received: 21 April 2016

Accepted: 11 July 2016

Published: 05 August 2016

DOI: https://doi.org/10.1038/srep31011

Yukihiro Miwa, Yusuke Hoshino, Chiho Shoda, Xiaoyan Jiang, Kazuo Tsubota Toshihide Kurihara Neurochemistry International (2019) Comments

By submitting a comment you agree to abide by our Terms and Community Guidelines. If you find something abusive or that does not comply with our terms or guidelines please flag it as inappropriate.