- •An Organ of Exquisite Perfection
- •Optical Path
- •Retinal Photoreception
- •Photoreception Optics
- •Photoreception Biochemistry
- •Membrane Voltages
- •Blind Spot
- •Retinal Pathways
- •Through Pathway
- •Receptive Fields
- •Lateral Pathway
- •Retinal Ganglion Cells
- •Retinal Glia
- •References
- •Development of the Foveal Specialization
- •Introduction
- •Foveal Development
- •Specification of Foveal Location
- •Formation of a Rod-Free Zone
- •Cones, Ganglion Cells, and Initial Pit Formation
- •Deep Foveal Pit Formation
- •Foveal Hypoplasia
- •Conclusions and Perspectives
- •Acknowledgments
- •References
- •An Update on the Regulation of Rod Photoreceptor Development
- •Introduction
- •Brief Overview of Retinal Development and Early Stages of Rod Photoreceptor Differentiation
- •Transcription Factors
- •Basic Helix-Loop-Helix Genes
- •Nuclear Receptors
- •Retinoic Acid/Retinoic Acid Receptors
- •Wnt/Frizzled Pathway
- •Taurine
- •Ciliary Neurotrophic Factor/Leukemia Inhibitory Factor/Pleiotrophin/Signal Transducer and Activators of Transcription 3/SOCS
- •Conclusions and Future Prospects
- •References
- •Introduction
- •Retinal Adhesion
- •Physiology of Retinal Adhesion
- •Molecular Mechanisms of Retinal Adhesion
- •Significance of Retinal Adhesion for Retinal Function
- •Photoreceptor Outer Segment Renewal
- •Physiology of Outer Segment Disk Assembly and Disk Shedding
- •Physiology of RPE Engulfment of Shed Outer Segment Fragments
- •Molecular Mechanisms of Shedding and RPE Phagocytosis
- •Significance of Photoreceptor Outer Segment Renewal for Retinal Function
- •Perspective
- •Acknowledgments
- •References
- •Molecular Biology of IRBP and Its Role in the Visual Cycle
- •Introduction
- •IRBP Protein Studies
- •IRBP Null Mice
- •IRBP Induces Experimental Autoimmune Uveitis
- •IRBP Expression During Development
- •Variability in IRBP Expression
- •Molecular Biology of IRBP
- •IRBP Genomic Cloning
- •Evolution of IRBP
- •Identification of DNA cis-Acting Controlling Elements: In Vitro and In Vivo Experiments
- •Transcription Factors and their Role in the Control of IRBP Expression
- •Rx/rax Transcription Factor
- •NrL Transcription Factor
- •Crx Transcription Factor
- •OTX2 Transcription Factor
- •Transgenic Mice
- •Repressors of IRBP Gene Expression
- •Summary and Conjecture
- •Acknowledgments
- •References
- •Regulation of Photoresponses by Phosphorylation
- •Introduction
- •Cone-Specific Kinase, GRK7
- •Protein Kinase C
- •Cyclin-Dependent Kinase
- •Tyrosine Kinases
- •Protein Phosphatases
- •Conclusion
- •References
- •The cGMP Signaling Pathway in Retinal Photoreceptors and the Central Role of Photoreceptor Phosphodiesterase (PDE6)
- •Regulation of Intracellular cGMP Levels in Photoreceptor Cells
- •Downstream Targets of cGMP Action in Photoreceptor Cells
- •cGMP-Dependent Protein Kinase
- •Cyclic Nucleotide-Gated Ion Channels
- •PDE6 Is a High-Affinity cGMP-Binding Protein
- •Compartmentation of cGMP Signaling in Photoreceptor Outer Segments
- •Physiology of the Photoreceptor Response to Light
- •Biochemical Cascade of Visual Excitation
- •Central Components of the cGMP Signaling Pathway
- •Termination and Adaptation of the Light Response
- •Deactivation of Rhodopsin
- •Deactivation of Transducin
- •Deactivation of PDE6
- •Activation of GC
- •Regulation of the CNG Ion Channel
- •Photoreceptor PDE (PDE6) Structure and Function
- •The Cyclic Nucleotide Phosphodiesterase Superfamily
- •Subunit Composition of Rod and Cone PDE6 Holoenzyme
- •Catalytic Subunit
- •Regulatory GAF Domain
- •Catalytic Domain
- •C-Terminal Prenylation
- •PDE6 Has Evolved to Meet the Special Demands of the Central Effector of Visual Transduction
- •PDE6 Regulation
- •Transducin Activation of Rod PDE6 During Visual Excitation
- •Functions of the Regulatory cGMP-Binding GAF Domains of PDE6
- •Potential PDE6 Regulatory Binding Proteins
- •Glutamic Acid-Rich Protein 2
- •Conclusions
- •Acknowledgments
- •References
- •Rhodopsin Structure, Function, and Involvement in Retinitis Pigmentosa
- •Introduction
- •Historical Perspective
- •Rhodopsin, Localization, and Signaling
- •Dark State and Activation
- •Structural Analysis
- •Electron Cryomicroscopy and Crystal Structure
- •Nuclear Magnetic Resonance
- •Cysteine Mutagenesis and Electron Paramagnetic Resonance
- •Other Approaches
- •Retinitis Pigmentosa
- •Transmembrane RP Rhodopsin Mutants
- •Cytoplasmic RP Rhodopsin Mutants
- •Intradiskal RP Rhodopsin Mutants
- •Implications of Receptor Misfolding
- •Nongenetic Contributions to RP
- •Conclusion
- •References
- •Multiple Signaling Pathways Govern Calcium Homeostasis in Photoreceptor Inner Segments
- •Introduction
- •Overview of Ca2+ Regulation in the Inner Segment
- •Voltage-Operated Calcium Channels Play a Central Role in Inner Segment Calcium Regulation
- •Ca2+ Channels in Rods and Cones
- •Photoreceptor Malfunction and Degeneration
- •Therapeutic Strategies
- •Development
- •Acknowledgments
- •References
- •The Transduction Channels of Rod and Cone Photoreceptors
- •The Role of CNG Channels in Photoreceptor Physiology
- •The Activation Phase of the Light Response
- •Recovery After a Light Stimulus and Adaptation to Continuous Illumination
- •CNG Channels in the Synaptic Transmission of Cone Photoreceptors
- •The Molecular Composition of CNG Channels
- •The Basic Activation Properties of CNG Channels
- •Transmembrane Topology and Functional Domains
- •The Cyclic-Nucleotide-Binding Domain
- •The Amino Terminal Domain and Modulation by Calmodulin
- •The P Region
- •The GARP Domain of CNGB1
- •Modulation by Phosphorylation and All-trans Retinal
- •Synthesis, Maturation, and Targeting of CNG Channels
- •Visual Dysfunction Caused by Mutant CNG Channel Genes
- •References
- •Appendix
- •Visual Dysfunction Caused by Mutant CNG Channel Genes
- •Mutations in CNGA1 and CNGB1 Associated with Retinitis Pigmentosa
- •Mutations in CNGA3 and CNGB3 Associated with Cone Dysfunction
- •References
- •Rhodopsins in Drosophila Color Vision
- •Introduction
- •Anatomy and Molecular Aspects of Color-Sensitive Opsins in the Drosophila Eye
- •Structure of the Drosophila Eye: Ommatidia, Photoreceptors, and Rhodopsins
- •Molecular Genetics and Evolution of Rh5 and Rh6
- •Development and Patterning of Rhodopsins for Drosophila Color Vision
- •Mutually Exclusive Rhodopsin Expression
- •Transcription Factors Specify Outer from Inner Photoreceptors and Distinguish R7 from R8
- •A Stochastic Decision Induces Rhodopsins in R7 Photoreceptor
- •A Bistable Feedback Loop Specifies R8 Photoreceptor Subtype and Expression of Rh5 and Rh6
- •Comparison Between Mammalian and Drosophila Color Vision Rhodopsins
- •Human Color-Sensitive Opsins
- •Conclusion
- •References
- •INAD Signaling Complex of Drosophila Photoreceptors
- •Introduction
- •Identification of the INAD Signaling Complex
- •Function of the INAD Signaling Complex
- •Information Transfer From Rhodopsin to the Signaling Complex BY the Visual G Protein
- •Signaling Complexes in Vertebrate Photoreceptor Cells
- •Acknowledgments
- •References
- •Visual Signal Processing in the Inner Retina
- •Introduction
- •Visual Information is First Processed in the OPL
- •Bipolar Cells form Parallel Pathways and Provide Excitatory Input to the IPL
- •Functional Stratification of the IPL
- •ON and OFF Response Stratification
- •Sustained and Transient Response Stratification
- •Synaptic Mechanisms Shape Excitatory Signals in the IPL
- •Glutamate Release Is Tonic and Graded
- •Transporters Terminate Excitatory Signaling to Ganglion Cells
- •Postsynaptic Glutamate Receptor Properties Shape Ganglion Cell Excitation
- •Modulating Glutamate Release Shapes Excitatory Responses
- •Amacrine Cells Mediate Inhibition in the IPL
- •Presynaptic Inhibition
- •Asymmetric Presynaptic Inhibition
- •Presynaptic Inhibition Is Filtered by GABA Receptor Properties
- •Presynaptic Inhibition May Be Shaped by Transmitter Release Differences
- •Glycine, the Other Inhibitory Transmitter
- •Parallel Ganglion Cell Output Pathways
- •Ganglion Cells Encode Color Information
- •Directional-Selective Ganglion Cells
- •Intrinsically Photosensitive Ganglion Cells
- •Conclusions
- •References
- •Human Cone Spectral Sensitivities and Color Vision Deficiencies
- •Introduction
- •Overview
- •Transduction
- •Univariance, Monochromacy, Dichromacy, and Trichromacy
- •Trichromacy and Color-Matching Functions
- •Cone Spectral Sensitivities
- •Introduction
- •Cone Spectral Sensitivity Measurements
- •From Cone Spectral Sensitivities to Color-Matching Functions
- •Other Factors That Influence Spectral Sensitivity
- •Lens Pigment
- •Macular Pigment
- •Photopigment Optical Density
- •Changes with Eccentricity
- •Congenital Color Vision Deficiencies
- •Protan and Deutan Defects
- •Protanopia and Deuteranopia
- •Photopigment Variability and Protanomaly and Deuteranomaly
- •Tritanopia
- •Monochromacies
- •Cone Monochromacies
- •Rod Monochromacy
- •Conclusions
- •Acknowledgment
- •References
- •Luminous Efficiency Functions
- •Introduction
- •The Need for Luminous Efficiency
- •Psychophysical Measures of Luminous Efficiency
- •Factors that Influence Luminous Efficiency
- •Scotopic (Rod) Luminous Efficiency Function
- •Introduction
- •Univariance
- •International Standard
- •Photopic (Cone) Luminous Efficiency Function
- •Introduction
- •International Standards
- •Other Photopic (Nonadditive) Luminous Efficiency Functions
- •Mesopic (Rod-Cone) Luminous Efficiency Functions
- •Introduction
- •Models of Mesopic Luminous Efficiency
- •International Standard
- •Individual Differences Influencing Luminous Efficiency
- •Attenuation of Spectral Light by the Lens and Other Ocular Media
- •Attenuation of Spectral Light by the Macular Pigment
- •Optical Densities of the Photopigments
- •Relative Numbers of L and M Cones
- •Cone Pigment Polymorphisms
- •Directional Sensitivity
- •Variations in the Contribution of Chromatic Channels
- •Conclusions
- •References
- •Cone Pigments and Vision in the Mouse
- •Introduction
- •Prevalence and Spatial Distribution of Mouse Cones
- •Mouse Strain Variations
- •Mouse Cone Pigments
- •Cone Pigment Spectra
- •Evolution and Spectral Tuning of Mouse Cone Pigments
- •Regional Distribution of Mouse Cone Pigments
- •Expression of Mouse Cone Pigments
- •Cone Signal Pathways in the Mouse Retina
- •Cone-Based Vision in Mice
- •Assessment Techniques
- •Spectral Sensitivity
- •Spatial and Temporal Sensitivity
- •Color Vision
- •Targeted Deletions of Rods or Cones
- •Addition of New Cone Pigments
- •Mouse and Human Cone Vision
- •Acknowledgment
- •References
- •Multifocal Oscillatory Potentials of the Human Retina
- •Introduction
- •Recording Techniques
- •Underlying Mechanisms
- •The Influence of age and Gender
- •Disease-Related Changes
- •Origins of Single Potentials
- •Dichromats
- •Congenital Stationary Night Blindness
- •Topographical Alterations
- •Diabetes
- •Retinal Vessel Occlusion
- •Glaucoma
- •General Alterations
- •Vigabatrin Treatment
- •Conclusion
- •References
- •The Aging of the Retina
- •Introduction
- •Morphological Alterations
- •Neural Changes
- •Retinal Pigment Epithelium and Lipofuscin Formation
- •Bruch’s Membrane and Choroid
- •Retinal Function Changes
- •Age-Related Macular Disease
- •Conclusions
- •References
- •Aging of the Retinal Pigment Epithelium
- •Introduction
- •Aging Changes In the Fundus
- •Age-Related Changes In RPE Morphology
- •Melanosomes
- •Lipofuscin
- •Pigment Complexes
- •Mitochondria
- •Bruch’s Membrane
- •Functional Consequences of RPE Cell Aging
- •Phagocytic Load
- •The Effect of Lipofuscin on the RPE
- •Melanosomes
- •Antioxidant Capacity of the RPE
- •Lysosomal Enzyme Activity
- •Mitochondrial Damage in the RPE
- •Bruch’s Membrane Aging
- •Oxidative Stress and RPE Aging
- •The Relationship Between Aging and Retinal Pathologies
- •Summary and Conclusions
- •References
- •Visual Transduction and Age-Related Changes in Lipofuscin
- •Introduction: What is Lipofuscin?
- •Lipofuscin of the Retinal Pigment Epithelium
- •Composition of RPE Lipofuscin
- •Fluorescence Properties of RPE Lipofuscin
- •A2E as a Marker of Lipofuscin Accumulation
- •Factors Affecting Accumulation of RPE Lipofuscin
- •Phagocytosis and Autophagy
- •Role of Lysosomal Degradation
- •Role of Oxidative Stress
- •Role of Phototransduction in Accumulation of RPE Lipofuscin
- •Transient Buildup of All-trans Retinal in Photoreceptor Outer Segments as a Critical Factor for Lipofuscin Formation
- •Inhibition of the Retinoid Cycle Inhibits Lipofuscin Accumulation
- •Role of Exposure of the Retina to Light
- •Other Factors Contributing to Accelerated Accumulation of RPE Lipofuscin
- •A Hypothetical Scenario of Biogenesis of RPE Lipofuscin
- •Effects of Lipofuscin on RPE Function and Viability
- •Photoreactivity of RPE Lipofuscin
- •Toxicity of RPE Lipofuscin
- •Effects of Lipofuscin Components and Oxidative Stress in the RPE on Proinflammatory and Angiogenic Signaling
- •Approaches to Diminish Lipofuscin Accumulation or Lipofuscin-Induced Damage
- •Conclusions
- •References
- •A Nonspecific System Provides Nonphotic Information for the Biological Clock
- •Introduction
- •Nonphotic Information
- •Nonspecific Systems
- •Ascending Reticular-Activating System
- •Orexin/Hypocretin Projection
- •Intergeniculate Leaflet of the Thalamus
- •Anatomy
- •The Pharmacology of the IGL
- •Chronobiology
- •The Electrophysiology of the IGL
- •IGL as an Integrator of Photic and Nonphotic Information
- •Conclusions
- •References
- •The Circadian Clock: Physiology, Genes, and Disease
- •Introduction
- •Circadian Rhythms in Physiology and Behavior
- •Circadian Rhythms in Visual Function
- •Entrainment
- •Anatomy
- •The Suprachiasmatic Nucleus
- •Inputs to the SCN
- •Peripheral Oscillators
- •A Clock in the Eye
- •Oscillators Outside the Nervous System
- •Clock Genes
- •Human Implications
- •Summary
- •References
280 |
Huber and Meyer |
ACKNOWLEDGMENTS
We wish to thank J. Pfannstiel and I. Huber for critical comments on the manuscript. Our work is supported by grants from the Deutsche Forschungsgemeinschaft (Hu 839/2-4), the German-Israel-Foundation (GIF), and the Hertie-Foundation.
REFERENCES
1.Lamb, T. D. (1996). Gain and kinetics of activation in the G-protein cascade of phototransduction. Proc. Natl. Acad. Sci. U. S. A. 93, 566–570.
2.Stryer, L. (1986). Cyclic GMP cascade of vision. Annu. Rev. Neurosci. 9, 87–119.
3.Hardie, R. C., Raghu, P. (2001). Visual transduction in Drosophila. Nature 413, 186–193.
4.Montell, C. (1999). Visual transduction in Drosophila. Annu. Rev. Cell Dev. Biol. 15, 231–268.
5.Koutalos, Y., Yau, K. W. (1996). Regulation of sensitivity in vertebrate rod photoreceptors by calcium. Trends Neurosci. 19, 73–81.
6.Wu, C. F., Pak, W. L. (1975). Quantal basis of photoreceptor spectral sensitivity of Drosophila melanogaster. J. Gen. Physiol. 66, 149–168.
7.Baylor, D. A., Lamb, T. D., Yau, K. W. (1979). Responses of retinal rods to single photons. J. Physiol. 288, 613–634.
8.Tsunoda, S., Sierralta, J., Zuker, C. S. (1998). Specificity in signaling pathways: assembly into multimolecular signaling complexes. Curr. Opin. Genet. Dev. 8, 419–422.
9.Ranganathan, R., Harris, G. L., Stevens, C. F., Zuker, C. S. (1991). A Drosophila mutant defective in extracellular calcium-dependent photoreceptor deactivation and rapid desensitization. Nature 354, 230–232.
10.Zuker, C. S. (1996). The biology of vision of Drosophila. Proc. Natl. Acad. Sci. U. S. A. 93, 571–576.
11.Minke, B., Parnas, M. (2006). Insights on TRP channels from in vivo studies in Drosophila. Annu. Rev. Physiol. 68, 649–684.
12.Minke, B., Hardie, R. C. (2000). Genetic dissection of Drosophila phototransduction. In: Handbook of biological physics, Volume 3: molecular mechanisms in visual transduction (Stavenga, D., DeGrip, W. J., Pugh, E. N., Jr., eds.), pp. 449–525. Elsevier, Amsterdam.
13.Pak, W. L., Leung, H. T. (2003). Genetic approaches to visual transduction in Drosophila melanogaster. Receptors Channels 9, 149–167.
14.Minke, B., Cook, B. (2002). TRP channel proteins and signal transduction. Physiol. Rev. 82, 429–472.
15.Paulsen, R., Bähner, M., Huber, A., Schillo, M., Schulz, S., Wottrich, R., Bentrop, J. (2001). The molecular design of a visual cascade: Molecular stages of phototransduction in Drosophila. In: Vision: the approach of biophysics and neurosciences (Musio, C., ed.), pp. 41–59. World Scientific, Singapore.
16.Tsunoda, S., Zuker, C. S. (1999). The organization of INAD-signaling complexes by a multivalent PDZ domain protein in Drosophila photoreceptor cells ensures sensitivity and speed of signaling. Cell Calcium 26, 165–171.
17.Paulsen, R., Bähner, M., Bentrop, J., Schillo, M., Schulz, S., Huber, A. (2001). The molecular design of a visual cascade: assembly of the Drosophila phototransduction pathway into a supramolecular signaling complex. In: Vision: the approach of biophysics and neurosciences (Musio, C., ed.), pp. 60–73. World Scientific, Singapore.
18.Montell, C. (1998). TRP trapped in fly signaling web. Curr. Opin. Neurobiol. 8, 389–397.
19.Huber, A. (2001). Scaffolding proteins organize multimolecular protein complexes for sensory signal transduction. Eur. J. Neurosci. 14, 769–776.
20.Ranganathan, R., Ross, E. M. (1997). PDZ domain proteins: scaffolds for signaling complexes. Curr. Biol. 7, R770–R773.
INAD Signaling Complex |
281 |
21.Zuker, C. S., Cowman, A. F., Rubin, G. M. (1985). Isolation and structure of a rhodopsin gene from D. melanogaster. Cell 40, 851–858.
22.O’Tousa, J. E., Baehr, W., Martin, R. L., Hirsh, J., Pak, W. L., Applebury, M. L. (1985). The Drosophila ninaE gene encodes an opsin. Cell 40, 839–850.
23.Gehring, W. J. (2002). The genetic control of eye development and its implications for the evolution of the various eye-types. Int. J. Dev. Biol. 46, 65–73.
24.Nakagawa, M., Iwasa, T., Kikkawa, S., Tsuda, M., Ebrey, T. G. (1999). How vertebrate and invertebrate visual pigments differ in their mechanism of photoactivation. Proc. Natl. Acad. Sci. U. S. A. 96, 6189–6192.
25.Bentrop, J., Paulsen, R. (2003). Invertebrate rhodopsins. In: Photoreceptors and light signalling (Batschauer, A., ed.), pp. 40–76. Royal Society of Chemistry, Cambridge, UK.
26.Chyb, S., Raghu, P., Hardie, R. C. (1999). Polyunsaturated fatty acids activate the Drosophila light-sensitive channels TRP and TRPL. Nature 397, 255–259.
27.Pak, W. L., Grossfield, J., Arnold, K. S. (1970). Mutants of the visual pathway of Drosophila melanogaster. Nature 227, 518–520.
28.Pak, W. L. (1979). Study of photoreceptor function using Drosophila mutants. In: Neurogenetics: genetic approaches to the nervous system (Breakefield, X., ed.), pp. 67–99. Elsevier, Amsterdam.
29.Bloomquist, B. T., Shortridge, R. D., Schneuwly, S., Perdew, M., Montell, C., Steller, H., Rubin, G., Pak, W. L. (1988). Isolation of a putative phospholipase C gene of Drosophila, norpA, and its role in phototransduction. Cell 54, 723–733.
30.Shieh, B. H., Niemeyer, B. (1995). A novel protein encoded by the InaD gene regulates recovery of visual transduction in Drosophila. Neuron 14, 201–210.
31.Tsunoda, S., Sierralta, J., Sun, Y., Bodner, R., Suzuki, E., Becker, A., Socolich, M., Zuker, C. S. (1997). A multivalent PDZ-domain protein assembles signalling complexes in a G-protein- coupled cascade. Nature 388, 243–249.
32.Shieh, B. H., Zhu, M. Y. (1996). Regulation of the TRP Ca2+ channel by INAD in Drosophila photoreceptors. Neuron 16, 991–998.
33.Huber, A., Sander, P., Gobert, A., Bahner, M., Hermann, R., Paulsen, R. (1996). The transient receptor potential protein (Trp), a putative store-operated Ca2+ channel essential for phosphoinositide-mediated photoreception, forms a signaling complex with NorpA, InaC and InaD. EMBO J. 15, 7036–7045.
34.Huber, A., Sander, P., Paulsen, R. (1996). Phosphorylation of the InaD gene product, a photoreceptor membrane protein required for recovery of visual excitation. J. Biol. Chem. 271, 11710–11717.
35.Chevesich, J., Kreuz, A. J., Montell, C. (1997). Requirement for the PDZ domain protein, INAD, for localization of the TRP store-operated channel to a signaling complex. Neuron 18, 95–105.
36.Wes, P. D., Xu, X. Z., Li, H. S., Chien, F., Doberstein, S. K., Montell, C. (1999). Termination of phototransduction requires binding of the NINAC myosin III and the PDZ protein INAD. Nat. Neurosci. 2, 447–453.
37.Xu, X. Z., Choudhury, A., Li, X., Montell, C. (1998). Coordination of an array of signaling proteins through homoand heteromeric interactions between PDZ domains and target proteins. J. Cell Biol. 142, 545–555.
38.Doyle, D. A., Lee, A., Lewis, J., Kim, E., Sheng, M., MacKinnon, R. (1996). Crystal structures of a complexed and peptide-free membrane protein-binding domain: molecular basis of peptide recognition by PDZ. Cell 85, 1067–1076.
39.Morais-Cabral, J. H., Petosa, C., Sutcliffe, M. J., Raza, S., Byron, O., Poy, F., Marfatia, S. M., Chishti, A. H., Liddington, R. C. (1996). Crystal structure of a PDZ domain. Nature 382, 649–652.
282 |
Huber and Meyer |
40.Hung, A. Y., Sheng, M. (2002). PDZ domains: structural modules for protein complex assembly. J. Biol. Chem. 277, 5699–5702.
41.Harris, B. Z., Lim, W. A. (2001). Mechanism and role of PDZ domains in signaling complex assembly. J. Cell Sci. 114, 3219–3231.
42.Songyang, Z., Fanning, A. S., Fu, C., Xu, J., Marfatia, S. M., Chishti, A. H., Crompton, A., Chan, A. C., Anderson, J. M., Cantley, L. C. (1997). Recognition of unique carboxyl-termi- nal motifs by distinct PDZ domains. Science 275, 73–77.
43.Stricker, N. L., Christopherson, K. S., Yi, B. A., Schatz, P. J., Raab, R. W., Dawes, G., Bassett, D. E., Jr., Bredt, D. S., Li, M. (1997). PDZ domain of neuronal nitric oxide synthase recognizes novel C-terminal peptide sequences. Nat. Biotechnol. 15, 336–342.
44.Maximov, A., Sudhof, T. C., Bezprozvanny, I. (1999). Association of neuronal calcium channels with modular adaptor proteins. J. Biol. Chem. 274, 24453–24456.
45.Kimple, M. E., Siderovski, D. P., Sondek, J. (2001). Functional relevance of the disulfide-linked complex of the N-terminal PDZ domain of InaD with NorpA. EMBO J. 20, 4414–4422.
46.Adamski, F. M., Zhu, M. Y., Bahiraei, F., Shieh, B. H. (1998). Interaction of eye protein kinase C and INAD in Drosophila. Localization of binding domains and electrophysiological characterization of a loss of association in transgenic flies. J. Biol. Chem. 273, 17713– 17719.
47.van Huizen, R., Miller, K., Chen, D. M., Li, Y., Lai, Z. C., Raab, R. W., Stark, W. S., Shortridge, R. D., Li, M. (1998). Two distantly positioned PDZ domains mediate multivalent INADphospholipase C interactions essential for G protein-coupled signaling. EMBO J. 17, 2285–2297.
48.Georgiev, P., Garcia-Murillas, I., Ulahannan, D., Hardie, R. C., Raghu, P. (2005). Functional INAD complexes are required to mediate degeneration in photoreceptors of the Drosophila rdgA mutant. J. Cell Sci. 118, 1373–1384.
49.Li, H. S., Montell, C. (2000). TRP and the PDZ protein, INAD, form the core complex required for retention of the signalplex in Drosophila photoreceptor cells. J. Cell Biol. 150, 1411–1421.
50.Tsunoda, S., Sun, Y., Suzuki, E., Zuker, C. (2001). Independent anchoring and assembly mechanisms of INAD signaling complexes in Drosophila photoreceptors. J. Neurosci. 21, 150–158.
51.Chorna-Ornan, I., Tzarfaty, V., Ankri-Eliahoo, G., Joel-Almagor, T., Meyer, N. E., Huber, A., Payre, F., Minke, B. (2005). Light-regulated interaction of Dmoesin with TRP and TRPL channels is required for maintenance of photoreceptors. J. Cell Biol. 171, 143–152.
52.Schulz, S., Huber, A., Schwab, K., Paulsen, R. (1999). A novel Gγ isolated from Drosophila constitutes a visual G protein γ subunit of the fly compound eye. J. Biol. Chem. 274, 37605–37610.
53.Yarfitz, S. L., Running, D. J., Froelick, G., Colley, N. J., Hurley, J. B. (1994). In situ assay of light-stimulated G protein activity in Drosophila photoreceptor G protein beta mutants. J. Biol. Chem. 269, 30340–30344.
54.Kosloff, M., Elia, N., Joel-Almagor, T., Timberg, R., Zars, T. D., Hyde, D. R., Minke, B., Selinger, Z. (2003). Regulation of light-dependent Gq alpha translocation and morphological changes in fly photoreceptors. EMBO J. 22, 459–468.
55.Cronin, M. A., Diao, F., Tsunoda, S. (2004). Light-dependent subcellular translocation of Gqalpha in Drosophila photoreceptors is facilitated by the photoreceptor-specific myosin III NINAC. J. Cell Sci. 117, 4797–4806.
56.Lee, S. J., Xu, H., Kang, L. W., Amzel, L. M., Montell, C. (2003). Light adaptation through phosphoinositide-regulated translocation of Drosophila visual arrestin. Neuron 39, 121–132.
INAD Signaling Complex |
283 |
57.Bähner, M., Frechter, S., Da Silva, N., Minke, B., Paulsen, R., Huber, A. (2002). Lightregulated subcellular translocation of Drosophila TRPL channels induces long-term adaptation and modifies the light-induced current. Neuron 34, 83–93.
58.Shieh, B. H., Zhu, M. Y., Lee, J. K., Kelly, I. M., Bahiraei, F. (1997). Association of INAD with NORPA is essential for controlled activation and deactivation of Drosophila phototransduction in vivo. Proc. Natl. Acad. Sci. U. S. A. 94, 12682–12687.
59.Henderson, S. R., Reuss, H., Hardie, R. C. (2000). Single photon responses in Drosophila photoreceptors and their regulation by Ca2+. J. Physiol. (Lond.) 524, 179–194.
60.Huber, A., Sander, P., Bahner, M., Paulsen, R. (1998). The TRP Ca2+ channel assembled in a signaling complex by the PDZ domain protein INAD is phosphorylated through the interaction with protein kinase C (ePKC). FEBS Lett. 425, 317–322.
61.Liu, M., Parker, L. L., Wadzinski, B. E., Shieh, B. H. (2000). Reversible phosphorylation of the signal transduction complex in Drosophila photoreceptors. J. Biol. Chem. 275, 12194–12199.
62.Popescu, D. C., Ham, A. J., Shieh, B. H. (2006). Scaffolding protein INAD regulates deactivation of vision by promoting phosphorylation of transient receptor potential by eye protein kinase C in Drosophila. J. Neurosci. 26, 8570–8577.
63.Bähner, M., Sander, P., Paulsen, R., Huber, A. (2000). The visual G protein of fly photore-
ceptors interacts with the PDZ domain assembled INAD signaling complex via direct binding of activated Gαq to phospholipase Cβ. J. Biol. Chem. 275, 2901–2904.
64.Scott, K., Becker, A., Sun, Y., Hardy, R., Zuker, C. (1995). Gq alpha protein function in vivo: genetic dissection of its role in photoreceptor cell physiology. Neuron 15, 919–927.
65.Scott, K., Zuker, C. S. (1998). Assembly of the Drosophila phototransduction cascade into a signalling complex shapes elementary responses. Nature 395, 805–808.
66.Hardie, R. C., Martin, F., Cochrane, G. W., Juusola, M., Georgiev, P., Raghu, P. (2002). Molecular basis of amplification in Drosophila phototransduction: Roles for G protein, phospholipase C, and diacylglycerol kinase. Neuron 36, 689–701.
67.Baylor, D. A., Matthews, G., Yau, K. W. (1980). Two components of electrical dark noise in toad retinal rod outer segments. J. Physiol. 309, 591–621.
68.Elia, N., Frechter, S., Gedi, Y., Minke, B., Selinger, Z. (2005). Excess of Gβe over Gqαe in vivo prevents dark, spontaneous activity of Drosophila photoreceptors. J. Cell Biol. 171, 517–526.
69.Cook, B., Bar-Yaacov, M., Cohen, B., Goldstein, R. E., Paroush, Z., Selinger, Z., Minke, B. (2000). Phospholipase C and termination of G-protein-mediated signalling in vivo. Nat. Cell Biol. 2, 296–301.
70.Molday, R. S. (1996). Calmodulin regulation of cyclic-nucleotide-gated channels. Curr. Opin. Neurobiol. 6, 445–452.
71.Körschen, H. G., Beyermann, M., Muller, F., Heck, M., Vantler, M., Koch, K. W., Kellner, R., Wolfrum, U., Bode, C., Hofmann, K. P., Kaupp, U. B. (1999). Interaction of glutamic- acid-rich proteins with the cGMP signalling pathway in rod photoreceptors. Nature 400, 761–766.
72.Poetsch, A., Molday, L. L., Molday, R. S. (2001). The cGMP-gated channel and related glutamic acid-rich proteins interact with peripherin-2 at the rim region of rod photoreceptor disc membranes. J. Biol. Chem. 276, 48009–48016.
73.Molday, R. S., Molday, L. L. (1998). Molecular properties of the cGMP-gated channel of rod photoreceptors. Vision Res. 38, 1315–1323.
74.Bauer, P. J., Drechsler, M. (1992). Association of cyclic GMP-gated channels and Na(+)- Ca(2+)-K+ exchangers in bovine retinal rod outer segment plasma membranes. J. Physiol. 451, 109–131.
284 |
Huber and Meyer |
75.Schwarzer, A., Kim, T. S., Hagen, V., Molday, R. S., Bauer, P. J. (1997). The Na/Ca-K exchanger of rod photoreceptor exists as dimer in the plasma membrane. Biochemistry. 36, 13667–13676.
76.Schwarzer, A., Schauf, H., Bauer, P. J. (2000). Binding of the cGMP-gated channel to the Na/Ca-K exchanger in rod photoreceptors. J. Biol. Chem. 275, 13448–13454.
77.Boesze-Battaglia, K., Lamba, O. P., Napoli, A. A., Jr., Sinha, S., Guo, Y. (1998). Fusion between retinal rod outer segment membranes and model membranes: a role for photoreceptor peripherin/rds. Biochemistry 37, 9477–9487.
