The fundamental role of the light receptor rhodopsin in visual function and photoreceptor cell development has been widely studied. Proper trafficking of rhodopsin to the photoreceptor membrane is of great importance. In human, mutations in rhodopsin involving its intracellular mislocalization, are the most frequent cause of autosomal dominant Retinitis Pigmentosa, a degenerative retinal pathology characterized by progressive blindness. Drosophila is widely used as an animal model in visual and retinal degeneration research. So far, little is known about the requirements for proper rhodopsin targeting in Drosophila.
Different truncated fly-rhodopsin Rh1 variants were expressed in the eyes of Drosophila and their localization was analyzed in vivo or by immunofluorescence. A mutant lacking the last 23 amino acids was found to properly localize in the rhabdomeres, the light-sensing organelle of the photoreceptor cells. This constitutes a major difference to trafficking in vertebrates, which involves a conserved QVxPA motif at the very C-terminus. Further truncations of Rh1 indicated that proper localization requires the last amino acid residues of a region called helix 8 following directly the last transmembrane domain. Interestingly, the very C-terminus of invertebrate visual rhodopsins is extremely variable but helix 8 shows conserved amino acid residues that are not conserved in vertebrate homologs.
Despite impressive similarities in the folding and photoactivation of vertebrate and invertebrate visual rhodopsins, a striking difference exists between mammalian and fly rhodopsins in their requirements for proper targeting. Most importantly, the distal part of helix 8 plays a central role in invertebrates. Since the last amino acid residues of helix 8 are dispensable for rhodopsin folding and function, we propose that this domain participates in the recognition of targeting factors involved in transport to the rhabdomeres.
Citation: Kock I, Bulgakova NA, Knust E, Sinning I, Panneels V (2009) Targeting of Drosophila Rhodopsin Requires Helix 8 but Not the Distal C-Terminus. PLoS ONE 4(7): e6101. doi:10.1371/journal.pone.0006101
Editor: Karl-Wilhelm Koch, University of Oldenburg, Germany
Received: April 14, 2009; Accepted: May 29, 2009; Published: July 2, 2009
Copyright: © 2009 Kock et al. This is an open-access article distributed under the terms of the Creative Commons Attribution License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original author and source are credited.
Funding: This work was supported by the European Community Specific Targeted Research Project grant IMPS (FP6-2003-LifeSciHealth 513770)to I.S. and by the European Commission [HEALTH-F2-2008-200234] to E.K. The funders had no role in study design, data collection and analysis, decision to publish, or preparation of the manuscript.
Competing interests: The authors have declared that no competing interests exist.
G protein-coupled receptors (GPCRs) represent the largest family of integral membrane proteins and are the main targets for drug development. They transmit a large variety of extracellular signals to the cell by activating different G proteins. The light receptor rhodopsin is still the best studied GPCR, serving as a prototype, due to its role in vision, but also – historically - due to its abundance in the photoreceptor cell membrane. The three-dimensional structure of endogenous bovine rhodopsin was determined already 10 years ago and served as the basis for understanding also the activation mechanism of GPCRs . Since then, progress with the structure determination of GPCRs was hampered by the low abundance of most GPCRs in their natural membranes and problems with stabilization. Recently the structure of a recombinant bovine rhodopsin expressed in insect cells was determined  as well as two structures from the β1 and β2-adrenergic receptors, again from recombinant material , . The latter ones were stabilized by different means including fusion proteins, antibody fragments and stabilizing mutations. We established a heterologous system for the overexpression of G protein-coupled receptors (GPCRs) in the eyes of transgenic flies . This system offers a number of advantages compared to conventional eukaryotic expression systems including its low costs and the high quality and homogeneity of the expressed proteins . Ectopic expression of recombinant GPCRs in transgenic Drosophila obtained by classical transposition into the genome of fly embryos was driven by an eye-specific promoter element in the photoreceptor cells. Containing microvillar rhabdomeric membranes endogenously filled with rhodopsin, these cells are ideally suited to yield functional GPCRs, as we have exemplarily demonstrated by expression, purification and reconstitution of a metabotropic glutamate receptor able to bind its ligand. Interestingly, by extending this study to a larger number of membrane proteins, we now found that some proteins e.g. the mammalian glutamate receptor, mGluR5, are not spontaneously targeted to the rhabdomeres, but are distributed in other non-ER membranous compartments (data not shown). These findings prompted us to study the molecular mechanisms driving the targeting of the most abundant rhabdomeric protein, the GPCR-prototype rhodopsin.
Faultless transport of rhodopsin from the photoreceptor cell body to the light sensitive membranous compartment of the eye is indispensable for proper visual function and eye development , . In human, rhodopsin mutations accounting for its intracellular mislocalization are the most frequent cause of autosomal dominant Retinitis Pigmentosa (RP) –, a degenerative retinal pathology characterized by progressive blindness. The most severe forms of RP are provoked by mutations clustered in the rhodopsin C-terminal QVxPA motif , which is conserved among vertebrates and has been shown to comprise a binding surface for transport-associated proteins , . Deletion or alteration of this motif induced trafficking impairment in both in vitro systems and animal models, the latter one accompanied by photoreceptor cell death, displaying its very important role for transport to the membranous rod outer segment (ROS) –.
In Drosophila, rhodopsin is not only essential for visual responses, but also plays a major role during photoreceptor cell development, being indispensable for the formation and maintenance of its own compartment, the rhabdomere , –. The rhabdomere consists of a highly pleated array of microvilli, formed by the apical membrane, which harbors the proteins of the phototransduction signaling cascade. Vesicular transport of rhodopsin to this light-sensitive organelle is known to take place from the trans-Golgi network (TGN) along the actin filamentous rhabdomere terminal web (involving the motorprotein MyoV ). However, the precise mechanism of rhodopsin trafficking to the rhabdomere remains elusive, and no distinct targeting signal has so far been identified in its amino acid sequence. In both vertebrates and invertebrates the C-terminus has been shown to act as a binding platform for various factors associated with signal transduction , . In example, termination of the light-response involves phosphorylation of a conserved serine-rich region in the C-terminus of rhodopsins and binding of arrestin followed by internalization of the complex. As a specific criterion of Class I GPCRs, the C-terminus of rhodopsin comprises a membrane anchored region containing an amphipathic helix (helix 8) and one or more palmitoylated cystein residues, followed by a flexible polar region. In vertebrate rhodopsins this polar region contains the thoroughly investigated QVxPA motif –,  required for effective targeting to the ROS. Given the importance of this motif, it is surprising to note that it is not conserved among invertebrates.
Here we show that major differences exist concerning the requirements to properly target vertebrate or invertebrate rhodopsins. The extreme C-terminus of Drosophila rhodopsin is dispensable, but the adjacent amphipathic region, helix 8, is crucial for correct localization of the receptor and intact eye morphology. In invertebrate rhabdomeric rhodopsins this region contains conserved amino acid residues, which are absent in vertebrate homologs. Helix 8 might therefore act as a binding domain for targeting factors involved in transport to the rhabdomeres.
Results and Discussion
The comparison of the C-terminal sequences of vertebrate and invertebrate rhodopsin shows that the QVxPA motif is not conserved in invertebrates, which show a significant variability in length and amino acid composition of their extreme C-termini (Fig. 1a). To determine the role of the C-terminal region in the targeting of the fly rhodopsin, we expressed several GFP-fused C-terminally truncated Drosophila rhodopsin Rh1 mutants (Fig. 1b–c) in the photoreceptor cells of transgenic flies and studied their ability to reach the rhabdomeres.
Figure 1. Analysis of the rhodopsin C-terminal region.
(a) Sequence alignment of the C-terminus from different species shows that the QVxPA motif of vertebrate rhodopsin is not conserved in invertebrate homologs. Bos.tau: Bos Taurus; Hom.sap: Homo sapiens; Tod.pac: Todarodes pacificus (squid); Pro.cla: Procambarus clarkii (crayfish); Dro.mel: Drosophila melanogaster. Alignment was done with ClustalW2 (EMBL-EBI). Numbers designate amino acid positions. “*” indicates identical (dark grey), “:” conserved (light grey) and “.” semi-conserved amino acid residues with respect to all investigated species. Helix 8 deduced from the structures of bovine and squid rhodopsin , ,  is denoted by a continuous black rectangle, QVxPA motif by a dashed black rectangle. “//” indicates position of residues discarded in the representation. (b+c) Schematic representation of Drosophila rhodopsin Rh1 variants used in this study. Numbers indicate amino acid positions. Putative helix 8 is denoted by a black box and the last amino acid of respective truncation mutants by colored circles (b) or rectangles (c) (blue: RhΔctΔH8, orange: Rhcc, green: RhLAL, red: RhΔct). Putative palmitoylation sites are illustrated by dashed lines linking the cystein residues to the membrane. Abbr. fl: full-length; nt: N-terminus; H8: helix 8.doi:10.1371/journal.pone.0006101.g001
We first removed the last 23 polar amino acids of Rh1 (RhΔct) and generated a transgenic fly expressing a truncated rhodopsin variant still containing the amphipathic helix 8 and a putative palmitoylation site. The flies were analyzed using three complementary techniques. Direct in vivo analysis of intact eyes and isolated ommatidia revealed strong fluorescence of rhabdomeres (Fig. 2a), as found in flies expressing GFP-fused wildtype rhodopsin , . Colocalization of RhΔct with F-Actin seen by immunofluorescence on ommatidia cross sections, confirmed its rhabdomeric localization (Fig. 2b). This leads to the conclusion that in contrast to its vertebrate counterparts, Drosophila rhodopsin does not require its flexible C-terminus for targeting to the light-sensitive organelle. Interestingly, in a different experimental context, other groups also showed a similar localization of the slightly longer Rh1Δ356 construct, which was left uncommented, but supports these findings , .
Figure 2. The C-terminally truncated Drosophila rhodopsin RhΔct localizes to the rhabdomeres.
(a) Direct in vivo confocal fluorescence microscopy on the intact eye (left) and isolated ommatidia (right) of adult flies expressing GFP-fused RhΔct reveals a rhabdomeric localization. (b) Optical cross sections of eyes stained with antibodies against GFP and Stardust (Sdt) show localization of the transgene-encoded protein (green) and stalk membrane (red) respectively. Phalloidin highlights F-Actin-rich rhabdomeres (blue). Merged picture displays extensive colocalization (in turquoise) of the rhodopsin truncation-mutant (green) with F-Actin (blue).doi:10.1371/journal.pone.0006101.g002
Additional removal of helix 8 (RhΔctΔH8 mutant) led to impaired transport of the receptor and a profound alteration of the rhabdomeric structure (Fig. 3). Analysis of both intact eyes and isolated ommatidia showed cytoplasmic accumulation of the protein (Fig. 3a), which was specified endoplasmic reticulum (ER)-based by its colocalization with KDEL in immunofluorescence (Fig. 3b). As ER-retention might be due to misfolding of the receptor , we also analyzed a slightly longer Rh1 variant, RhLAL, corresponding to a truncation mutant of bovine rhodopsin able to bind retinal and couple to transducin, indicating its proper folding , . Preserving the proximal part of helix 8 (Fig. 4), in these flies the rhabdomeric structure was present but RhLAL did not colocalize with the rhabdomere marker F-Actin as seen in optical cross sections (Fig. 4b). The shortest Rh1 mutant properly targeted to rhabdomeres (RhCC) comprises the entire helix 8 (Fig. S1), showing that the distal part of helix 8 is crucial. It is noteworthy that flies expressing the RhCC or RhLAL variants develop smaller eyes compared to the RhΔct flies, which showed a normal morphology (Fig. S1) as well as a perfect fluorescent pseudopupil (data not shown). As the RhCC variant localized in rhabdomeres, it implies that the eye phenotype was not due to a dramatic alteration in rhodopsin trafficking. The palmitoylation site downstream of helix 8 has been shown to be dispensable for the trafficking of both Drosophila and vertebrate rhodopsins ,  and therefore the proper targeting of RhCC is most likely due to the essential role of helix 8 in the targeting of Rh1.
Figure 3. Helix 8 is required for rhabdomere targeting of rhodopsin.
(a) Direct in vivo confocal fluorescence microscopy on intact eye (left) and isolated ommatidia (right) of adult flies expressing GFP-fused RhΔctΔH8, lacking the helix 8 region, shows an extrarhabdomeric distribution-pattern of the truncation-mutant. (b) Optical cross sections, stained with antibodies against GFP and KDEL to show localization of the transgene (green) and ER (red), respectively, reveal its colocalization (orange) with the KDEL antibody, indicating ER-based distribution of the protein. Phalloidin highlights F-Actin-rich rhabdomeres (blue).doi:10.1371/journal.pone.0006101.g003
Figure 4. The distal part of Helix 8 is crucial for rhabdomere targeting of rhodopsin.
Confocal fluorescence microscopy on intact eye (left) and optical cross sections of an eye expressing RhLAL (right), lacking the distal part of helix 8, shows extrarhabdomeric distribution of the rhodopsin variant. The GFP-tagged protein accumulates at the rhabdomere base (in green) and partially colocalizes (in orange) with KDEL, indicating ER-based distribution of the protein (right panel). Optical cross sections were stained with antibodies against GFP and KDEL to show localization of the transgene (green) and ER (red) respectively. Phalloidin highlights F-Actin-rich rhabdomeres (blue).doi:10.1371/journal.pone.0006101.g004
Analysis of invertebrate opsin sequences showed that rhabdomeric opsins like Rh1 (Fig. S2A) and to a lower extent ciliary opsins, that are homologous to the family of vertebrate visual opsins (Fig. S2B) show high conservation in the proximal part of helix 8 (see the PKY/FR motif). They contain a conserved proline marking the end of helix 8. In the structure of the squid rhodopsin , , the two conserved prolines induce kinks delimiting helix 8 and their conservation in rhabdomeric opsins suggests common structural features. It is interesting to see the high similarity in the structures of squid rhabdomeric and bovine ciliary rhodopsins despite their low sequence homology . The difference in sequence cannot be attributed to divergence of vertebrate and invertebrate rhodopsins because earlier animal phyla like cnidarians possess both ciliary and rhabdomeric opsins . Moreover the invertebrates honeybee and annelid Platynereis have visual rhabdomeric opsins but also non-visual light-detecting opsins that are orthologous to vertebrate ciliary visual opsins . It seems curious that recombinant bovine rhodopsin is properly targeted to the rhabdomeres of a transgenic Drosophila  since it contains the QVxPA motif but not the residues in helix 8 of Drosophila Rh1 which are conserved in rhabdomeric opsins. This may simply indicate that the targeting machinery of Drosophila melanogaster can also recognize a targeting motif in the bovine ciliary rhodopsin. Conversely, mammals have a rhabdomeric-like opsin in the retina, melanopsin, playing a role in non-visual responses to light , . Melanopsin contains the conserved PKY/FR motif as well as the proline terminating helix 8 as described here for Drosophila. A closer inspection of rhabdomeric visual opsins from insects shows that helix 8 is highly conserved (see the PKYRxxLxxR/K motif), but not the very C-terminus of the protein (Fig. S2C). While the proximal part of helix 8 is important in signal transduction in vertebrates ,  and also possibly in invertebrates, in invertebrates the distal part of helix 8 might play a role in the trafficking process. Whether this involves structural requirements e.g. helix formation still needs to be shown.
In summary, our data show that helix 8 of Drosophila rhodopsin and not the very C-terminus is essential for proper targeting to the rhabdomere. In contrast, vertebrate rhodopsin shows mislocalization already in the absence of the C-terminal QVxPA motif , –. Mazelova et al. recently identified an Arf4 GTPase based targeting complex specifically recognizing the VxPx consensus and thus allowing transport of vertebrate rhodopsin to the ciliary ROS . The consensus sequence is also found in other ciliary membrane proteins, but is absent in rhabdomeric rhodopsin homologs. Together with our findings, this strongly suggests major differences in the targeting of the two rhodopsin families to their respective membranes. There may be a different mechanism responsible for selection and packaging of the rhabdomeric homologs. If during targeting they also interact with a GTPase, they might use helix 8 instead of the C-terminus. Based on our data it is tempting to speculate that this interaction involves conserved residues present at the distal part of helix 8. Ciliary vertebrate and rhabdomeric invertebrate visual rhodopsins are known to activate different G proteins, involve distinct signaling cascades and possess an individual structural fingerprint , , , [revised in 44]. We have shown that they also differ in their targeting sequences. In the future further thorough investigations are needed to understand the exact underlying mechanisms in invertebrates.
The Drosophila rhodopsin coding sequence was amplified from a w1118 Drosophila cDNA library (kindly provided by F. Weber, BZH) by PCR using specific primers, and ligated in the pUAST vector (a kind gift from JC Desplan, New York) between EcoRI and NotI restriction sites. Rhodopsin truncation mutants were generated by PCR from this template and cloned alike in pUAST. They encode the following rhodopsin amino acids: RhΔct: 1–350, Rhcc 1–347, RhLAL 1–340, RhΔctΔH8: 1–333 (see Fig. 1). All of the rhodopsin constructs contain a linker sequence encoding three glycine residues upstream of the NotI restriction site itself coding for three alanines. The nucleotide sequence of eGFP flanked by NotI and XbaI restriction sites was inserted downstream of the rhodopsin and linker sequences. All nucleotide sequences were verified by DNA sequencing.
Construction and Keeping of Transgenic Flies
Constructs described above were transformed into Drosophila w1118 embryos by the Vanedis Drosophila injection service (Norway) by classical P-element transposition. Target-gene expression was driven specifically in the eyes by the Glass Multimer Reporter (GMR)-Gal4 (GMR-Gal4 flies were a kind gift from G. Merdes, ZMBH, Heidelberg) and verified by Western blot analysis using an anti-GFP antibody (Biovision), diluted 1:2000. All flies were kept at 25° or room temperature on a 12 h day/12 h night cycle.
Confocal Fluorescence Microscopy
All images were acquired using a Zeiss LSM 510 confocal microscope mounted on an Axiovert 200 inverted microscope equipped with an argon laser beam. Image processing was performed with Adobe Photoshop CS3 according to the guidelines for proper digital image handling .
In vivo Microscopy of intact Eyes
Flies were fixed to object slides through a transthoracic needle oriented so that the eyes are placed facing upward. Pictures were taken with a 40× objective lens immersed in oil covering the cornea of the fly. A minimum of eight flies of each genotype were analyzed.
Isolation of ommatidia and direct in vivo Microscopy
At least 10 fly heads of each genotype were bisected, transferred into Schneider cell medium (Gibco) and prepared under a binocular. Using fine needles, retinas were freed from surrounding tissue and fragmented until appropriate in size. Samples were protected by cover slips and instantly analyzed using a 63× objective (NA 0.55).
To verify the in vivo data and determine the precise intracellular distribution of the rhodopsin variants, we checked for colocalization with organelle-specific antibodies in immunofluorescence microscopy. Optical cross sections and immunohistochemistry were performed as previously described . The following primary antibodies were used: mouse anti-KDEL (Stressgen) 1:500 marking the ER, mouse anti-Stardust (Sdt) 1:400 labeling the stalk membrane that is a part of apical membrane adjacent (basally) to the rhabdomere  and rabbit anti-GFP (Invitrogen) 1:500. Detection was performed by the following corresponding secondary fluorescent antibodies: Cy3 conjugated anti-mouse (Dianova) 1:200 and Cy2 conjugated anti-rabbit (Dianova) 1:200. F-Actin of rhabdomeres was stained by Alexa Fluor 660 phalloidin (Molecular Probes) 1:40.
Eye phenotype of the trangenic fly RhCC is not correlated with a defect in rhodopsin trafficking. Eye morphology of one-day old transgenic flies expressing RhΔct (Rh1, 1–350, panel d), RhCC (Rh1, 1–347, panel h) or RhLAL (Rh1, 1–340, panel l)) was analysed in parallel with the localization of the truncated Rh1 transgene-encoded protein in isolated ommatidia. Typical bright field- and fluorescent images of isolated ommatidia obtained by confocal microscopy (objective 60x) are shown in panels [c, g, k] and [a–b, e–f, i–j], respectively. Although both RhΔct and RhCC proteins were localized in rhabdomeres (see panel a–b and e–f, respectively), the fly expressing RhΔct had a normal eye morphology (panel d) while the RhCC fly displays a smaller eye (panel h).
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The conserved amino acid residues flanking helix 8 in rhabdomeric opsins are not conserved in ciliary opsins. (a) Sequence alignment of C-terminal regions of rhabdomeric opsins from various phyla of invertebrates using ClustalW2 (EBI, EMBL): Drosophila melanogaster (Dro.mel., Arthropoda), Apis mellifera (Api.mel., Arthropoda), Daphnia pulex (Dap.pul., Crustacean), Schistosoma mansoni (Schi.man., Platyhelminthe), Todarodes pacificus (Tod.pac., Mollusca), Platynereis dumerilii (Plat.dum., Annelida), Lottia gigantea (Lot.gig., Mollusca). Partial sequences are presented from the ultraconserved NPxxY GPCR-consensus motif to the end, except if interrupted (//). Identical (*), conserved (:) and semi-conserved (.) residues are labeled at the bottom of the alignment. The sequence corresponding to helix 8 in squid rhodopsin (Tod.pac.) is underlined. (b) Sequence alignment of C-terminal regions of ciliary opsins from invertebrates: some invertebrates, like the bee and some annelids, have both ciliary and rhabdomeric opsins. Here, the ciliary opsins of Apis mellifera (Bee) (Api.mel., Arthropoda) and Platynereis dumerilii (Plat.dum., Annelida) are aligned in comparison with the earliest animal phylum possessing complex eyes Cladonema radiatum (Cla.rad., Cnidaria). The Drosophila melanogaster (Dro.mel., Arthropoda) sequence is shown in light grey for comparison (the conserved proline is underlined). (c) Sequence alignment of C-terminal regions of 23 rhabdomeric opsins from different insects: Drosophila melanogaster (Dro.me1, Dro.me2 to Dro.me6 are the Rh1 (ninaE), Rh2 to Rh6 opsins, respectively), Calliphora erythrocephala (Cal.ery), Papilio xuthus (Pap.xu1 and Pap.xu2 are Rh2 and Rh5, respectively), Pieris rapae (Pie.rap), Manduca sexta (Man.se1 and Man.se2 are the products of Manop1 and Manop2 genes, respectively), Vanessa cardui (Van.car), Apis mellifera (Api.me1 and Api.me2 are LWSRh1 and LWSRh2 (long wavelength sensitive opsins), respectively and Api.me3 is an UV-sensitive opsin), Cataglyphis bombycinus (Cat.bo1 and Cat.bo2 are a Rh1 and a short wavelength-sensitive opsin, respectively), Tribolium castaneum (Tri.cas), Schistocerca gregaria (Sch.gre), Pediculus humanus (Ped.hum), Camponotus abdominalis (Cam.abd) and Rhodnius prolixus (Rho.pro). Identical (*), conserved (:) and semi-conserved (.) residues are labeled at the bottom of the alignment. The sequence corresponding to helix 8 of Drosophila Rh1, deduced from the squid rhodopsin structure, is underlined.
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The authors thank D. Richter (Forschungszentrum, Karlsruhe, Germany) for technical advice and discussions, and S. Adrian for technical assistance.
Conceived and designed the experiments: IS VP. Performed the experiments: IK NAB VP. Analyzed the data: IK NAB EK IS VP. Contributed reagents/materials/analysis tools: NAB EK IS VP. Wrote the paper: IK IS VP.
- 1. Palczewski K, Kumasaka T, Hori T, Behnke CA, Motoshima H, et al. (2000) Crystal structure of rhodopsin: A G protein-coupled receptor. Science 289: 739–745.
- 2. Standfuss J, Xie G, Edwards PC, Burghammer M, Oprian DD, et al. (2007) Crystal structure of a thermally stable rhodopsin mutant. J Mol Biol 372: 1179–1188.
- 3. Cherezov V, Rosenbaum DM, Hanson MA, Rasmussen SG, Thian FS, et al. (2007) High-resolution crystal structure of an engineered human beta2-adrenergic G protein-coupled receptor. Science 318: 1258–1265.
- 4. Warne T, Serrano-Vega MJ, Baker JG, Moukhametzianov R, Edwards PC, et al. (2008) Structure of a beta1-adrenergic G-protein-coupled receptor. Nature 454: 486–491.
- 5. Eroglu C, Cronet P, Panneels V, Beaufils P, Sinning I (2002) Functional reconstitution of purified metabotropic glutamate receptor expressed in the fly eye. EMBO Rep 3: 491–496.
- 6. Humphries MM, Rancourt D, Farrar GJ, Kenna P, Hazel M, et al. (1997) Retinopathy induced in mice by targeted disruption of the rhodopsin gene. Nat Genet 15: 216–219.
- 7. Kumar JP, Ready DF (1995) Rhodopsin plays an essential structural role in Drosophila photoreceptor development. Development 121: 4359–4370.
- 8. Dryja TP, McGee TL, Hahn LB, Cowley GS, Olsson JE, et al. (1990) Mutations within the rhodopsin gene in patients with autosomal dominant retinitis pigmentosa. N Engl J Med 323: 1302–1307.
- 9. Dryja TP, McGee TL, Reichel E, Hahn LB, Cowley GS, et al. (1990) A point mutation of the rhodopsin gene in one form of retinitis pigmentosa. Nature 343: 364–366.
- 10. Colley NJ, Cassill JA, Baker EK, Zuker CS (1995) Defective intracellular transport is the molecular basis of rhodopsin-dependent dominant retinal degeneration. Proc Natl Acad Sci U S A 92: 3070–3074.
- 11. Berson EL, Rosner B, Weigel-DiFranco C, Dryja TP, Sandberg MA (2002) Disease progression in patients with dominant retinitis pigmentosa and rhodopsin mutations. Invest Ophthalmol Vis Sci 43: 3027–3036.
- 12. Tai AW, Chuang JZ, Bode C, Wolfrum U, Sung CH (1999) Rhodopsin's carboxy-terminal cytoplasmic tail acts as a membrane receptor for cytoplasmic dynein by binding to the dynein light chain Tctex-1. Cell 97: 877–887.
- 13. Deretic D, Williams AH, Ransom N, Morel V, Hargrave PA, et al. (2005) Rhodopsin C terminus, the site of mutations causing retinal disease, regulates trafficking by binding to ADP-ribosylation factor 4 (ARF4). Proc Natl Acad Sci U S A 102: 3301–3306.
- 14. Sung CH, Makino C, Baylor D, Nathans J (1994) A rhodopsin gene mutation responsible for autosomal dominant retinitis pigmentosa results in a protein that is defective in localization to the photoreceptor outer segment. J Neurosci 14: 5818–5833.
- 15. Deretic D, Schmerl S, Hargrave PA, Arendt A, McDowell JH (1998) Regulation of sorting and post-Golgi trafficking of rhodopsin by its C-terminal sequence QVS(A)PA. Proc Natl Acad Sci U S A 95: 10620–10625.
- 16. Tam BM, Moritz OL, Hurd LB, Papermaster DS (2000) Identification of an outer segment targeting signal in the COOH terminus of rhodopsin using transgenic Xenopus laevis. J Cell Biol 151: 1369–1380.
- 17. Washburn T, O'Tousa JE (1989) Molecular defects in Drosophila rhodopsin mutants. J Biol Chem 264: 15464–15466.
- 18. Leonard DS, Bowman VD, Ready DF, Pak WL (1992) Degeneration of photoreceptors in rhodopsin mutants of Drosophila. J Neurobiol 23: 605–626.
- 19. Ahmad ST, Natochin M, Artemyev NO, O'Tousa JE (2007) The Drosophila rhodopsin cytoplasmic tail domain is required for maintenance of rhabdomere structure. FASEB J 21: 449–455.
- 20. Li BX, Satoh AK, Ready DF (2007) Myosin V, Rab11, and dRip11 direct apical secretion and cellular morphogenesis in developing Drosophila photoreceptors. J Cell Biol 177: 659–669.
- 21. Wang T, Duan Y (2007) Chromophore channeling in the G-protein coupled receptor rhodopsin. J Am Chem Soc 129: 6970–6971.
- 22. Wensel TG (2008) Signal transducing membrane complexes of photoreceptor outer segments. Vision Res 48: 2052–2061.
- 23. Deretic D (1998) Post-Golgi trafficking of rhodopsin in retinal photoreceptors. Eye 12 ( Pt 3b): 526–530.
- 24. Pichaud F, Desplan C (2001) A new visualization approach for identifying mutations that affect differentiation and organization of the Drosophila ommatidia. Development 128: 815–826.
- 25. Sarfare S, Ahmad ST, Joyce MV, Boggess B, O'Tousa JE (2005) The Drosophila ninaG oxidoreductase acts in visual pigment chromophore production. J Biol Chem 280: 11895–11901.
- 26. Vinos J, Jalink K, Hardy RW, Britt SG, Zuker CS (1997) A G protein-coupled receptor phosphatase required for rhodopsin function. Science 277: 687–690.
- 27. Satoh AK, Ready DF (2005) Arrestin1 mediates light-dependent rhodopsin endocytosis and cell survival. Curr Biol 15: 1722–1733.
- 28. Weiss ER, Osawa S, Shi W, Dickerson CD (1994) Effects of carboxyl-terminal truncation on the stability and G protein-coupling activity of bovine rhodopsin. Biochemistry 33: 7587–7593.
- 29. Cai K, Klein-Seetharaman J, Farrens D, Zhang C, Altenbach C, et al. (1999) Single-cysteine substitution mutants at amino acid positions 306–321 in rhodopsin, the sequence between the cytoplasmic end of helix VII and the palmitoylation sites: sulfhydryl reactivity and transducin activation reveal a tertiary structure. Biochemistry 38: 7925–7930.
- 30. Bentrop J, Paulsen R (2003) Invertebrate rhodopsins. Photoreceptors and Light Signalling. pp. 40–76.
- 31. Wang Z, Wen XH, Ablonczy Z, Crouch RK, Makino CL, et al. (2005) Enhanced shutoff of phototransduction in transgenic mice expressing palmitoylation-deficient rhodopsin. J Biol Chem 280: 24293–24300.
- 32. Shimamura T, Hiraki K, Takahashi N, Hori T, Ago H, et al. (2008) Crystal structure of squid rhodopsin with intracellularly extended cytoplasmic region. J Biol Chem 283: 17753–17756.
- 33. Murakami M, Kouyama T (2008) Crystal structure of squid rhodopsin. Nature 453: 363–367.
- 34. Kozmik Z, Ruzickova J, Jonasova K, Matsumoto Y, Vopalensky P, et al. (2008) Assembly of the cnidarian camera-type eye from vertebrate-like components. Proc Natl Acad Sci U S A 105: 8989–8993.
- 35. Arendt D (2003) Evolution of eyes and photoreceptor cell types. Int J Dev Biol 47: 563–571.
- 36. Koyanagi M, Kubokawa K, Tsukamoto H, Shichida Y, Terakita A (2005) Cephalochordate melanopsin: evolutionary linkage between invertebrate visual cells and vertebrate photosensitive retinal ganglion cells. Curr Biol 15: 1065–1069.
- 37. Isoldi MC, Rollag MD, Castrucci AM, Provencio I (2005) Rhabdomeric phototransduction initiated by the vertebrate photopigment melanopsin. Proc Natl Acad Sci U S A 102: 1217–1221.
- 38. Lehmann N, Alexiev U, Fahmy K (2007) Linkage between the intramembrane H-bond network around aspartic acid 83 and the cytosolic environment of helix 8 in photoactivated rhodopsin. J Mol Biol 366: 1129–1141.
- 39. Altenbach C, Kusnetzow AK, Ernst OP, Hofmann KP, Hubbell WL (2008) High-resolution distance mapping in rhodopsin reveals the pattern of helix movement due to activation. Proc Natl Acad Sci U S A 105: 7439–7444.
- 40. Green ES, Menz MD, LaVail MM, Flannery JG (2000) Characterization of rhodopsin mis-sorting and constitutive activation in a transgenic rat model of retinitis pigmentosa. Invest Ophthalmol Vis Sci 41: 1546–1553.
- 41. Concepcion F, Mendez A, Chen J (2002) The carboxyl-terminal domain is essential for rhodopsin transport in rod photoreceptors. Vision Res 42: 417–426.
- 42. Lee ES, Flannery JG (2007) Transport of truncated rhodopsin and its effects on rod function and degeneration. Invest Ophthalmol Vis Sci 48: 2868–2876.
- 43. Mazelova J, Astuto-Gribble L, Inoue H, Tam BM, Schonteich E, et al. (2009) Ciliary targeting motif VxPx directs assembly of a trafficking module through Arf4. EMBO J 28: 183–192.
- 44. Hardie RC, Raghu P (2001) Visual transduction in Drosophila. Nature 413: 186–193.
- 45. Voie AM, Cohen S (1998) Germ-line transformation of Drosophila melanogaster. In cell biology: a laboratory handbook. pp. 510–517.
- 46. Rossner M, Yamada KM (2004) What's in a picture? The temptation of image manipulation. J Cell Biol 166: 11–15.
- 47. Richard M, Grawe F, Knust E (2006) DPATJ plays a role in retinal morphogenesis and protects against light-dependent degeneration of photoreceptor cells in the Drosophila eye. Dev Dyn 235: 895–907.
- 48. Berger S, Bulgakova NA, Grawe F, Johnson K, Knust E (2007) Unraveling the genetic complexity of Drosophila stardust during photoreceptor morphogenesis and prevention of light-induced degeneration. Genetics 176(4): 2189–200.