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Visual sensation in vertebrates is triggered when light strikes retinal photoreceptor cells causing photoisomerization of the rhodopsin chromophore 11-cis-retinal to all-trans-retinal. The regeneration of preillumination conditions of the photoreceptor cells requires formation of 11-cis-retinal in the adjacent retinal pigment epithelium (RPE). Using the intrinsic fluorescence of all-trans-retinyl esters, noninvasive two-photon microscopy revealed previously uncharacterized structures (6.9 ± 1.1 μm in length and 0.8 ± 0.2 μm in diameter) distinct from other cellular organelles, termed the retinyl ester storage particles (RESTs), or retinosomes. These structures form autonomous all-trans-retinyl ester-rich intracellular compartments distinct from other organelles and colocalize with adipose differentiation-related protein. As demonstrated by in vivo experiments using wild-type mice, the RESTs participate in 11-cis-retinal formation. RESTs accumulate in Rpe65−/− mice incapable of carrying out the enzymatic isomerization, and correspondingly, are absent in the eyes of Lrat−/− mice deficient in retinyl ester synthesis. These results indicate that RESTs located close to the RPE plasma membrane are essential components in 11-cis-retinal production.
Metabolic transformations of retinoids within the retinal photoreceptor and retinal pigment epithelium (RPE) are responsible for the production of the chromophore essential for vision, 11-cis-retinal (McBee et al., 2001). Within the RPE, all-trans-retinol (vitamin A), a product of photoisomerized and reduced 11-cis-retinal, is esterified with fatty acids in a reaction catalyzed by lecithin:retinol acyltransferase (LRAT; Fig. 1; Saari et al., 1993). LRAT was identified on the molecular level as a 25-kD protein (Ruiz et al., 1999) that is expressed in several tissues, including liver and the RPE (for review see McBee et al., 2000). All-trans-retinyl esters are intermediate compounds in a pathway (“retinoid cycle”) that recycles 11-cis-retinal, the chromophore of the visual pigments of rod and cone photoreceptors (for review see Bok, 1985; McBee et al., 2001). All-trans-retinyl esters have been suggested to be the substrate for a putative isomerohydrolase in the RPE (Rando, 1991) and for a retinyl ester hydrolase that produces all-trans-retinol, a substrate for the putative isomerase (for review see McBee et al., 2000). Regardless of the enzymatic pathway, 11-cis-retinol is produced, oxidized to 11-cis-retinal, and exported to the photoreceptors where it recombines with opsins to form 11-cis-retinylidene-opsins (rhodopsin, and cone pigments; Fig. 1; for review see Filipek et al., 2003).
Defects in the retinoid cycle may lead to blinding disorders, such as retinitis pigmentosa or macular degeneration (Rattner et al., 1999; Dryja, 2000; Baehr et al., 2003). Among these, the inherited early onset dystrophies are collectively called Leber congenital amaurosis (LCA). LCA is a group of genetically heterogeneous diseases that involves, among others, mutations in LRAT and RPE-specific 65-kD protein (RPE65) genes (Gu et al., 1997; Marlhens et al., 1997; Morimura et al., 1998; Perrault et al., 1999; Thompson et al., 2001). Animal models of these specific LCA were generated (Redmond et al., 1998; Batten et al., 2003) to address functional consequences of the targeted gene disruption on the retinoid metabolism. Recently, somatic gene therapy and pharmacological intervention were successful in restoration of vision in the dog and mouse animal models of LCA, respectively, with the nonfunctional RPE65 gene (Van Hooser et al., 2000, 2002; Acland et al., 2001).
Although several retinoid metabolites are generated during regeneration of 11-cis-retinal, only retinol and retinyl esters show a weak intrinsic fluorescence (excitation λ at ~320 nm; Sears and Kaplan, 1989; Garwin and Saari, 2000; Kuksa et al., 2003; Zipfel et al., 2003). Simultaneous absorption of two photons and excitation of intrinsic fluorophores, in conjunction with laser scanning fluorescence microscopy (Denk et al., 1990; Bennett et al., 1996), has been exploited to generate three-dimensional (3-D) temporal and spectral-resolved images of cells, tissues, or organs (Euler et al., 2002; Wang et al., 2003). Here, infrared two-photon microscopy was used to monitor changes in the distribution of vitamin A and its metabolites in the intact mouse eye without mechanical disruption of the essential close contacts between the photoreceptor and the RPE, photobleaching of rhodopsin, or photodamage to the tissue. The retinyl ester storage structures increased in the RPE of wild-type mice exposed to light or in an age-dependent manner in light- and dark-adapted Rpe65−/− mice incapable of carrying out the enzymatic isomerization, and they were absent in the eyes of Lrat−/− mice deficient in vitamin A. Thus, two-photon microscopy revealed changes in the retinyl ester pool in normal and pathological states in vivo, without disruption of the fragile RPE–retina interface.
Two-photon microscopy, with excitation at λ = 730 nm directly through the sclera of the dissected mouse eye, revealed a clear image of fluorescent compartments ~50 μm (390–545-nm emission; Fig. 2 A, red pseudocolor) and within ~1–40 μm (560–700-nm emission) from the surface of the sclera (Fig. 2 A, green pseudocolor). Taking advantage of the layered structure of the eye (Kolb et al., 2001), the two fluorescent compartments were localized within the RPE (red) and the sclera (green). Localization of these compartments was deduced based on morphological criteria, such as appropriate distances verified by histological sectioning (unpublished data), differences in the appearance of nuclei in each layer (Fig. 2 A, right column), and on the appearance of the capillaries in the choroid. RPE fluorescence in the unstained eyecup displayed unique elongated structures perpendicular to the cell layer with a length of 6.9 ± 1.1 μm, a diameter of 0.8 ± 0.2 μm, and frequency of 36.2 ± 2.2 per double-nuclei cells (n = 200; Fig. 2 B, a). 3-D projections of these fluorescent structures present in the RPE showed particular localization and remarkable symmetry (Video 1, available at http://www.jcb.org/cgi/content/full/jcb.200311079/DC1). Antibodies against RPE-dominant transmembrane 11-cis-retinol dehydrogenase (Fig. 2 B, b), membrane-associated RPE65 (Fig. 2 B, c), and soluble cellular retinaldehyde-binding protein (CRALBP; Fig. 2 B, d) confirmed the intracellular position of the autofluorescent structures. 3-D projections of these fluorescent structures (red) and anti-11-cis-retinol dehydrogenase immunostaining (green) in the RPE demonstrated that they did not colocalize (Video 2). Similarly, 3-D projections of these structures (red) and anti-RPE65 immunostaining (green) in the RPE showed that they are present in nonoverlapping cellular compartments (Video 3).
Bleaching of rhodopsin in the intact rod-dominant mouse eye led to time-dependent increase in fluorescence within the RPE layer with the half-time τ1/2 = 10 min (n = 3), without significant changes within the rod outer segments (ROSs; Fig. 2 C, top two left panels). The change paralleled a light-dependent increase in the formation of all-trans-retinol and all-trans-retinyl esters (τ1/2 = 10 min; n = 3) in the RPE as determined by normal phase HPLC (Fig. 2 C, bottom left; Van Hooser et al., 2002), suggesting these structures contain retinoids. The fluorescence signal localized specifically to these subcellular structures, which we termed retinyl ester storage particles (RESTs), or retinosomes. The fluorescence signal increase coincided with formation of all-trans-retinol/all-trans-retinyl esters (unpublished data). The results for a 60-min incubation in the dark are shown in Fig. 2 C (right). These data are consistent with earlier observations that the visual cycle does not proceed to the 11-cis-retinoid production in the dissected eyes and eyecups (Palczewski et al., 1999), and that under physiological temperature- and oxygen/carbonated-control conditions the reaction mostly proceeds to all-trans-retinyl ester formation (~65%; unpublished data). When the eyecups were incubated with a soluble complex of vitamin A ((2-hydroxypropyl)-β-cyclodextrin·all-trans-retinol), significant increases in fluorescence and all-trans-retinyl ester formation were observed in these structures (Fig. 2 D, b). The increases in the fluorescence intensity coincided with increases of the retinyl ester content (Fig. 2 D, c and d), strengthening the argument that these structures contain the fluorescent retinyl esters. No tissue damage was observed after two-photon excitation, as determined by the analysis of histological sections.
Fluorescent RESTs are not a part of Golgi (Fig. 3 a), mitochondria (Fig. 3 b), a majority of lysosomes (Fig. 3 c), the plasma membrane (Fig. 3 d), or the ER (Fig. 3 e). RESTs also did not colocalize with autofluorescent A2E, a component of lipofuscin, an age-related by-product of ROS phagocytosis by the RPE (Liu et al., 2000; unpublished data). NADH and NADPH were poorly excited at 730 nm and were not observed in our experiments, as demonstrated by the lack of mitochondrial fluorescence (see also Kuksa et al., 2003). The RESTs did not colocalize with peroxisomes, as visualized by immunofluorescence techniques with catalase, a marker of these organelles (unpublished data). However, using immunocytochemistry, we found that adipose differentiation-related protein (ADRP) colocalizes with the RESTs (Fig. 3 f). ADRP was shown previously to localize at the vicinity of the plasma membrane involved in the formation and stabilization of lipid droplets (Gao and Serrero, 1999; Targett-Adams et al., 2003).
Tangential sections of the RPE, analyzed by EM, showed that most of the mouse RPE contained two nuclei (Fig. 3, g and h), as observed in rats (Owaribe et al., 1988). Moreover, vacuole-like structures with translucent inclusions were often present close to the boundary of the cells (Fig. 3, g and h). After flash stimulation of rhodopsin (Fig. 3 g), the vacuole-like structures were more inflated compared with those kept in the dark (Fig. 3 h). The diameters of the structures were ~1 μm after flash stimulation (Fig. 3 i). Electron-dense vesicles observed throughout the cell were membrane inclusions (ingested ROS) or peroxisomes. The location, size, and frequency of the vacuole-like structures corresponded with RESTs observed by two-photon microscopy, suggesting that RESTs may incorporate retinyl esters, thereby increasing their volume.
If RESTs participate in production of 11-cis-retinal, no light-dependent changes in two-photon excited autofluorescence should be observed in the RPE of mice lacking a functional RPE65 gene, which is essential for chromophore regeneration (Redmond et al., 1998). Although the wild-type RPE increased their fluorescence intensity (arbitrary unit) from 0.56 ± 0.28 to 1.52 ± 0.56 after an intense 10-ms flash that bleached ~60% of the pigment (Fig. 4 A, a, b, and g), these changes were not observed in the RPE of Rpe65−/− mice (Fig. 4 A, c, d, and g). Consistently, the amounts of all-trans-retinyl esters increased from 71.4 ± 3.3 to 274.2 ± 32.4 pmol for wild-type mice, whereas for the eyes of Rpe65−/− mice the amount was 207.6 ± 19.5 pmol for pre-flash conditions and comparable to 192.3 ± 6.6 pmol post-flash (Fig. 4 A, g).
LRAT could be the enzyme essential for trapping retinoids from bleached photoreceptors and for removing them from the circulation (McBee et al., 2001). Hence, Lrat−/− mice were generated and analyzed (Batten et al., 2003). Total retinoid analyses revealed that the eyes of Lrat−/− mice contained residual amounts of retinoids (~8.3 pmol/eye in 4-wk-old mice) and no functional rhodopsin (Batten et al., 2003). For comparison, ~500 pmol retinoid/eye was present in the wild-type or Lrat+/− littermates, mostly in opsin-bound 11-cis-retinylidene form. Because only trace amounts of all-trans-retinol and retinyl esters were present in the RPE of Lrat−/− mice (Fig. 4 A, g; Batten et al., 2003), the RESTs are not formed (Fig. 4 A, e and f). No light-dependent changes in the retinoid levels as assayed by fluorescence or HPLC were observed in the eyes of Lrat−/− mice (Fig. 4 A, e–g).
In the RPE of Rpe65−/− mice, age-dependent increase in formation of lipid droplet-like structures filled with a translucent lipid-like substance was attributed to all-trans-retinyl ester accumulation (Van Hooser et al., 2002). Therefore, we investigated REST formation as a function of age in the RPE of Rpe65−/− mice. Here, a systematic increase of retinoids was observed with increasing age in the RPE of these mice (Fig. 4 B). The increase in RPE fluorescence intensity paralleled the increase in the all-trans-retinyl ester accumulation (Fig. 4 B, d) and formation of a spherical body, morphologically distinct from normal RESTs, within the RPE. These results provide the first direct evidence that the “oil-droplets” (Redmond et al., 1998) are formed, at least in part, from all-trans-retinyl esters.
To observe directly whether RESTs participate in the flow of retinoids, we extended our analyses to live mice. We acquired fluorescence images at the periphery of the retina directly through the sclera, using thoroughly dark-adapted and anesthetized mice (Fig. 5 A). After a light flash, the change in the fluorescence intensity of RESTs paralleled the formation of all-trans-retinyl esters in the RPE of those mice (Fig. 5 B). The retinyl ester pool peaked at 30 min (Fig. 5 B, b) and the regeneration of 11-cis-retinal is nearly completed within 60 min (Saari et al., 1998), corresponding to formation of 11-cis-retinal and disappearance of all-trans-retinal (Fig. 5 B, c). On light stimulation, the number of RESTs appeared to be similar as in the RPE of the dark-adapted mice, but their intensity increased significantly.
To test whether RESTs are essential for the isomerization process, we gavaged Lrat−/− mice with 9-cis-retinal, as described previously for Rpe65−/− mice (Van Hooser et al., 2002). 9-cis-retinal recombined with opsin, forming isorhodopsin, as demonstrated by the analysis of retinoids in the eye, UV-Vis spectroscopy of the detergent extract from the eye, and isolation of isorhodopsin by immunoaffinity chromatography (unpublished data). After bleach, 9-cis-retinal bound to opsin was converted to all-trans-retinal. Without formation of retinyl ester, and hence RESTs, all-trans-retinal/all-trans-retinol were quickly lost from the eye (Fig. 5 C). Accordingly, no formation of 11-cis-retinal (with different chromatographic and spectral properties from 9-cis-retinal) was observed. These results demonstrate that RESTs participate in retinoid storage and restoration of the chromophore after photobleaching.
Because ADRP colocalized with the RESTs (Fig. 3 f), we investigated whether its expression and localization is altered in genetically engineered mice that have enhanced accumulation of all-trans-retinyl esters or lack them entirely. The overaccumulation of all-trans-retinyl esters in the RPE of Rpe65−/− mice coincided with accumulation of ADRP in the RESTs as observed in the eyes of Rpe65−/− mice. In contrast, ADRP was present throughout the RPE cytoplasm of Lrat−/− mice lacking retinyl esters (Fig. 6, A and B). In the RPE cells of Lrat−/− mice, ADRP was expressed at lower levels (Fig. 6 B), which suggests that ADRP is a protein component of the RESTs.
Our aim was to use native and genetically modified mice in conjunction with microscopy, HPLC, and immunocytochemistry to understand mechanisms governing the retinoid cycle and visual transduction. Spectrally sensitive noninvasive two-photon microscopy in conjunction with genetically engineered mice lacking key components of the retinoid cycle was used to identify a novel structure in the RPE involved in the production of the visual chromophore, 11-cis-retinal. Two-photon microscopy permitted deep tissue penetration of infrared excitation light in anesthetized mice to monitor regeneration processes of rhodopsin without introducing external fluorophores. Our results revealed the existence of novel structures, RESTs (or retinosomes), that are critical to the formation of 11-cis-retinal.
In wild-type mice, all-trans-retinol exchanges rapidly between the blood and the RPE (Qtaishat et al., 2003). RESTs appear to be essential structures for retaining esterified vitamin A in the eye to support its utilization in formation of the chromophore for visual pigments. RESTs are also essential for trapping all-trans-retinol generated in photoreceptors, which must diffuse across the ECM separating ROSs and the RPE. Subcellular localization of these structures allows efficient trapping of all-trans-retinol from both the choroidal circulation and from photoreceptors after photoisomerization of rhodopsin's chromophore. This process is stalled in the RPE of Rpe65−/− mice (Redmond et al., 1998; Qtaishat et al., 2003) that overaccumulate all-trans-retinyl esters in aberrantly large RESTs (Fig. 4).
The flow of soluble retinoids in either free or protein-bound form is governed by the gradient generated by the conversion of 11-cis- and all-trans-retinol to insoluble all-trans-retinyl esters in the RPE and the conversion of 11-cis-retinal to 11-cis-retinylidene-opsin in rod photoreceptor cells (McBee et al., 2001). Hence, compartmentalization plays an essential role in driving energetically unfavorable chemical reactions through mass action (McBee et al., 2001). The all-trans-retinyl esters constitute a storage intermediate in the isomerization pathway from all-trans- to 11-cis-isomers (Rando, 1996). The isomerization proceeds through a reaction that involves an unidentified enzyme-retinol intermediate, or a specific subpopulation of all-trans-retinyl esters with properties that are distinct from the bulk of all-trans-retinyl esters (Stecher et al., 1999). All-trans-retinyl esters present in the RESTs and formed in situ on the internal membranes where LRAT resides may form two subpopulations, from which only one is used for the isomerization process directly.
Several molecular components involved in the 11-cis-retinal formation have been identified through biochemical and genetic approaches. RPE65 is thought to be involved in the delivery of all-trans-retinyl esters to the isomerization machinery by the virtue of specific binding of these esters (Gollapalli et al., 2003; Mata et al., 2004). Our analyses add a cell biological view for the formation of retinyl esters during the retinoid cycle. All-trans-retinol likely diffuses first to the ER, where the major fraction is converted to retinyl esters by the ER-localized LRAT. Our in vivo analysis demonstrates that the retinyl esters are next delivered to and stored in RESTs. Blocking the redistribution of all-trans-retinyl esters from RESTs resulted in aberrant accumulation of all-trans-retinyl esters in RESTs as observed in the RPE of Rpe65−/− mice. In photoreceptors of Lrat−/− mice regenerated with 9-cis-retinal, photoisomerization of isorhodopsin (9-cis-retinylidene-opsin) produced all-trans-retinoids, which could not be converted to 11-cis-retinal, hence formation of rhodopsin (11-cis-retinylidene-opsin) was not observed. Free all-trans-retinol could be quickly lost to the circulation, whereas all-trans-retinyl esters are essential in the retention of retinoids in the eye. This observation does not discard the possibility that all-trans-retinol is used directly by a putative isomerase, simply because all-trans-retinyl esters could be the starting substrate for the RPE65–hydrolase–isomerase complex indispensable in the production of 11-cis-retinol.
On average, between 20 and 40 ROSs project toward one RPE cell (for review see McBee et al., 2001). For efficient transfer of retinoid between the RPE and the photoreceptor cells, the retinoid-processing enzymes should be widely distributed throughout the cell as observed in this and previous reports (McBee et al., 2001; Haeseleer et al., 2002; Batten et al., 2003). Once the retinoids are esterified, they are trapped into RESTs (Fig. 7), which are composed of all-trans-retinyl esters and at least one additional protein component, ADRP. The formation of self-associating complexes of all-trans-retinyl esters (Li et al., 1996) could facilitate REST formation. Clustering of all-trans-retinyl esters may prevent diffusion of retinoids through the retina, and may circumvent overproduction of all-trans-retinoic acid, an agent known to cause cell differentiation and proliferation (Mangelsdorf et al., 1995), thus lowering overall toxicity. However, the symmetric nature of these structures and their intracellular distribution suggest that perhaps additional proteins are also involved. Interestingly, Liu et al. (2003) provided evidence that the lipid droplets in CHO K2 cells are metabolic organelles involved in membrane traffic, and that they contained ADRP as a major protein component of these structures termed adiposomes. It is tempting to speculate that ADRP could be an essential component of the lipid structures throughout the body.
Prior reports of myeloid bodies in the RPE have demonstrated that they vary in size during light adaptation (Tabor and Fisher, 1983; Abran and Dickson, 1992a,b; Dickson and Morrison, 1993; Cai and Dickson, 1994), suggesting possible involvement in the retinoid cycle. However, the appearance and location of the REST is different from the myeloid bodies, and the relationship between these two structures is unclear. Robison and Kuwabara (1977) observed accumulation of lipid inclusion droplets along the basal and lateral cell boundaries after injection of the substantial dose of all-trans-retinyl esters. In our experiments, the subcellular localization of the RESTs, a minor component of the RPE, and appearance of these structures differ from those previous observations. Most EM analyses were performed on radial sections of the eye, and hence it was difficult to provide quantitative results for the thin structures perpendicularly aligned to the RPE cell layer. A combination of EM and application of two-photon microscopy to study visual processes using the infrared laser for the excitation of the fluorophores opens a new way to detect and study the subcellular structures.
In summary, in this work we have used the power of noninvasive, spectrally sensitive two-photon microscopy in conjunction with genetically engineered mice lacking key components of the retinoid cycle to define a novel structure in the RPE, the RESTs (Fig. 7). Two-photon microscopy has unsurpassed potential to advance our understanding of normal physiological processes and to provide new insights into the pathology of many other eye diseases using suitable mouse models.
The University of Washington and University of Utah Animal Care Committees approved all of the procedures that used animal experiments. Animals were maintained in complete darkness, and all of the manipulations with animals, dissected eyes, or retinoids were performed under dim red light using a No. 1 Safelight filter (transmittance >560 nm; Kodak). The Balb/c mice were used as a wild type throughout the experiments. Rpe65−/− mice were obtained from Dr. M. Redmond (National Eye Institute, National Institutes of Health, Bethesda, MD). Lrat−/− mice were generated as recently described (Batten et al., 2003). Albino lines of Rpe65−/− and Lrat−/− mice were maintained in a mixed background of 129Sv, C57Bl/6, and Balb/c. Rpe65−/− mice were genotyped as described previously (Redmond et al., 1998). Mice were anesthetized by i.p. injection using 15 μl/g body weight of 6 mg/ml ketamine and 0.44 mg/ml xylazine diluted with 10 mM phosphate buffer, pH 7.2, containing 100 mM NaCl. The gavage experiments were performed on Lrat mice as described for Rpe65 mice in Van Hooser et al. (2002).
Two-photon excitation microscopy was performed using a confocal microscope (LSM 510 MP-NLO; Carl Zeiss MicroImaging, Inc.) with LSM510 software v3.0. Briefly, 76-MHz, 100-fs pulses of 730-nm light from a mode-locked Ti:Sapphire laser (Mira-900; Coherent) were focused on the sample by a Plan-Neofluar 40×/1.3 NA objective lens for ex vivo experiments and a Planapochromat 20×/0.75 NA lens for in vivo experiments (Carl Zeiss MicroImaging, Inc.). The intensity of the laser was measured at the back aperture of the objective lens and kept at ~3 mW for ex vivo analysis and ~5 mW for in vivo analysis. For 3-D imaging of RESTs in Fig. 1 B, the average power of the laser was kept at ~10 mW. Autofluorescence from the sample (390–545 nm) was collected by the objective, separated from the excitation light by a dichroic mirror, filtered to remove scattered excitation light, and directed to a photomultiplier tube detector. The objective lens was heated to 37°C by an air stream incubator. A temperature-controlled microscopic stage was installed on the microscope to maintain the reaction at 37°C. Fluorescent intensities reflected in pixel values were calculated by off-line analysis of the collected raw images (SCION image; Scion Co.). Fluorescent intensity was measured for the tangential sections of the RPE, and was averaged per pixel for randomly chosen areas (mean ± SD; n = 30 from three eyes) enclosing 100 × 100 pixels (~30 × 30 μm2 for Fig. 1 B and C and Fig. 3; 36 × 36 μm2 for Fig. 4). For separation of the cytoplasmic, nucleic, and REST responses (Fig. 1 B, right), fluorescent intensities were averaged for randomly chosen areas of 25 pixels (~2 μm2; n = 180 for three independent eyes). In Fig. 1 D, the RPE was exposed to 1.4 mM all-trans-retinol caged with 100 mM (2-hydroxypropyl)-β-cyclodextrin for 2 min, and was washed briefly with Ames medium (Sigma-Aldrich) for 3 min.
For ex vivo imaging, immediately after eye removal, mouse eyes or eyecups were located at the center of a glass-bottomed 35-mm dish and perfused with oxygenized (95% O2, 5% CO2) Ames medium at 37°C. For in vivo observation, an anesthetized mouse was laid on the temperature-controlled microscopic stage (at 37°C), and the right side of the eye was located on the microscopic cover glass (44-mm-diam, 0.16-mm thickness; Carl Zeiss MicroImaging, Inc.). In this way, the retina was imaged at the periphery by the laser penetrating through the sclera while the emission fluorescence was collected coming back to the microscopic objective lens. In case of a slight movement of the eye, the same area of the retina was traced using unique texture of the RPE cell layer formed by the randomly arranged single- and dual-nucleated RPE. In most experiments, thoroughly dark-adapted mice were exposed to an intense 10-ms flash that bleached ~60% of the pigment.
Retinoids were stored in N,N-dimethylformamide under argon at −80°C, and the concentrations were determined spectrophotometrically (Garwin and Saari, 2000). All retinoids were purified by normal phase HPLC (Ultrasphere-Si, 4.6 mm × 250 mm; Beckman Coulter) with 10% ethyl acetate/90% hexane at a flow rate of 1.4 ml/min (Van Hooser et al., 2000).
Eyecups were prepared by removing anterior segments and neural retinas from the isolated mouse eyes, and the exposed RPE was fixed with 4% PFA for 15 min at 37°C. Immunofluorescence detection of antigens by anti-RPE65 antibody (a gift of M. Redmond, National Eye Institute), anti-CRALBP antibody (a gift of J.C. Saari, University of Washington, Seattle, WA), anti-ADRP (Progen), and anti-11-cis-retinol dehydrogenase (Haeseleer et al., 2002) was performed as described previously (Haeseleer et al., 2002). Samples were incubated with the primary antibody for 1 h and for 30 min with the secondary antibody conjugated with Cy3 (Jackson ImmunoResearch Laboratories).
A number of fluorescent dyes (Molecular Probes, Inc.) were applied to the live RPE in the eyecup. Golgi apparatus was visualized by introducing 50 μM BODIPY® FL C5-ceramide. Two emission ranges were collected (500–530 nm for green pseudocolor and 560–700 nm for blue pseudocolor) from the fluorophore that had two emission peaks (515 nm and ~620 nm) by excitation at 488 nm. Mitochondria were visualized by 200 nM MitoTracker® Orange CMTMRos, and emissions from 560 to 700 nm were collected by excitation at 543 nm. Acidic organelles including lysosomes were visualized by 200 nM LysoTracker® Green DND-26, and the emission range from 500 to 550 nm was collected by excitation at 488 nm. For visualization of the plasma membrane, 1 mM FM 4-64 was applied to the RPE and emission was collected at ~650 nm (λex = 543 nm). DiOC6 dye was applied at 5 μg/ml to visualize the ER, and the emission was collected from 500 to 550 nm excited at 488 nm. A2E (green) was visualized by collecting emission from 565 to 615 nm by excitation at 488 nm. Fluorescent signals were covisualized with RESTs using a laser scanning microscope (LSM510; Carl Zeiss MicroImaging, Inc.) under appropriate filter configuration.
For figure preparation, Adobe Photoshop® 6.0 was used for adjustments of brightness and for color balance. 3-D reconstructed projections shown in Fig. 1 B and in the supplemental videos were generated using LSM510 software v3.0 (Carl Zeiss MicroImaging, Inc.).
Dark-adapted mice controls or dark-adapted mice exposed to an intense flash (10-ms duration) that bleached ~60% of the pigment were used for TEM. Photobleached mice were allowed to recover for 30 min to allow formation of retinyl esters. Mouse eyecups were primarily fixed by immersion in 2.5% glutaraldehyde and 1.6% PFA in 0.08 M Pipes, pH 7.4, containing 2% sucrose initially at RT for ~1 h, and then at 4°C for the remainder of 24 h (Van Hooser et al., 2002). The eyecups were then washed with 0.13 M sodium phosphate, pH 7.35, and secondarily fixed with 1% OsO4 in 0.1 M sodium phosphate, pH 7.35, for 1 h at RT. The eyecups were dehydrated through a methanol series and transitioned to the epoxy-embedding medium with propylene oxide. The eyecups were embedded for sectioning in Eponate 812. Ultrathin sections (60–70 nm) were stained with aqueous saturated uranium acetate and Reynold's formula lead citrate before survey and micrography with an electron microscope (model CM10; Philips).
Video 1 shows retinyl ester storage particles in the RPE cells. Three-dimensional projections of retinyl ester storage particles in the RPE cells. Video 2 shows covisualization of retinyl ester storage particles and 11-cis-retinol dehydrogenase. Three-dimensional projections of retinyl ester storage particles (red) and 11-cis-retinol dehydrogenase (green) in the RPE cells. Video 3 shows covisualization of retinyl ester storage particles and RPE65. Three-dimensional projections of retinyl ester storage particles (red) and RPE65 (green) in the RPE cells.
We would like to thank Drs V. Gerke, R. Rodieck, A. Polans, and A. Moise for insightful comments on the manuscript; Dr. M. Redmond for providing Rpe65−/− mice and anti-RPE65 antibody; Dr. J.C. Saari for anti-CRALBP antibody; and D. Possin for the EM analysis.
This research was supported by National Institutes of Health grants EY09339, EY13385, EY08123 (to W. Baehr), and DK53434 (to D.W. Piston); National Science Foundation grant DBI9871063 (to D.W. Piston); a grant from Research to Prevent Blindness, Inc. (RPB) to the Departments of Ophthalmology at the University of Washington and the University of Utah; the Stargardt and Retinal Eye Disease Fund; a grant from the Macular Vision Research Foundation (to W. Baehr); a Foundation for Fighting Blindness Center grant to the University of Utah; and a grant from the E.K. Bishop Foundation (to K. Palczewski). K. Palczewski and W. Baehr are RPB Senior Investigators.
The online version of this article includes supplemental material.
Abbreviations used in this paper: 3-D, three-dimensional; ADRP, adipose differentiation-related protein; CRALBP, cellular retinaldehyde-binding protein; LRAT, lecithin:retinol acyltransferase; REST, retinyl ester storage particle; ROS, rod outer segment; RPE, retinal pigment epithelium; RPE65, an RPE-specific 65-kD protein.