Molecular Vision 2019; 25:921-933
Received 08 August 2019 | Accepted 30 December 2019 | Published 31 December 2019
The first two authors contributed equally to the manuscript.
1Department of Human Anatomy, Histology and Embryology, School of Basic Medicine, Qingdao University, Qingdao266071, Shandong Province, China; 2State Key Laboratory Cultivation Base, Shandong Provincial Key Laboratory of Ophthalmology, Shandong Eye Institute, Shandong First Medical University & Shandong Academy of Medical Sciences, Qingdao, China
Correspondence to: Peng Chen, Department of Human Anatomy, Histology and Embryology, School of Basic Medicine, Qingdao University, 308 Ningxia Road, Qingdao 266071, China; Phone: (532) 8378-0061; FAX: (532) 83780081; Email: email@example.com.
Purpose: To elucidate the clinical phenotypes and pathogenesis of a novel missense mutation in guanylate cyclase activator A1A (GUCA1A) associated with autosomal dominant cone dystrophy (adCOD).
Methods: The members of a family with adCOD were clinically evaluated. Relevant genes were captured before being sequenced with targeted next-generation sequencing and confirmed with Sanger sequencing. Sequence analysis was made of the conservativeness of mutant residues. An enzyme-linked immunosorbent assay (ELISA) was implemented to detect the cyclic guanosine monophosphate (cGMP) concentration. Then limited protein hydrolysis and an electrophoresis shift were used to assess possible changes in the structure. Coimmunoprecipitation was employed to analyze the interaction between GCAP1 and retGC1. Immunofluorescence staining was performed to observe the colocalization of GCAP1 and retGC1 in human embryonic kidney (HEK)-293 cells.
Results: A pathogenic mutation in GUCA1A (c.431A>G, p.D144G, exon 5) was revealed in four generations of a family with adCOD. GUCA1A encodes guanylate cyclase activating protein 1 (GCAP1). D144, located in the EF4 loop involving calcium binding, was highly conserved in the species. GCAP1-D144G was more susceptible to hydrolysis, and the mobility of the D144G band became slower in the presence of Ca2+. At high Ca2+ concentrations, GCAP1-D144G stimulated retGC1 in the HEK-293 membrane to significantly increase intracellular cGMP protein concentrations. Compared with wild-type (WT) GCAP1, GCAP1-D144G had an increased interaction with retGC1, as detected in the coimmunoprecipitation assay.
Conclusions: The newly discovered missense mutation in GUCA1A (p.D144G) might lead to an imbalance of Ca2+ and cGMP homeostasis and eventually, cause a significant variation in adCOD.
Cone dystrophy (COD) and cone-rod dystrophy (CORD) are retinal diseases that can be inherited as dominant, recessive, or X-linked traits  but are mainly acquired through autosomal dominant (ad) inheritance. They are characterized by damage to vision, abnormal color vision, and varying degrees of nystagmus and photophobia in the early stage, followed by peripheral visual field loss and even blindness . CORD involves progressive loss of cone photoreceptor function followed by gradual loss of rod cell function, and it is usually accompanied by retinal degeneration . However, in hereditary progressive COD, only the cone function is impaired, with retinal degeneration limited to the central retina. Clinical phenotypes of COD have significant heterogeneity, so the performance of each patient in the same family can range from photoaversion to cone dystrophy.
Ten disease-causing genes (AIPL1-gene ID: 23746; OMIM: 604392; CRX-gene ID:1406; OMIM: 602225; GUCA1A-gene ID: 2978; OMIM: 600364; GUCY2D-gene ID: 3000; OMIM: 600179; PITPNM3-gene ID: 83394; OMIM: 608921; PROM1-gene ID: 8842; OMIM: 604365; PRPH2-gene ID: 83394; OMIM: 608921; RIMS1-gene ID: 22999; OMIM: 606629; SEMA4A-gene ID: 64218; OMIM: 607292, and UNC119-gene ID: 9094; OMIM: 604011) and four loci (CORD4-gene ID: 9094; OMIM: 604011;
CORD12-gene ID: 8842; OMIM: 604365; CORD17-gene ID: 101409267; OMIM: 615163, and RCD1-gene ID: 5953; OMIM: 180020) with unidentified genes have been found in adCOD and adCORD (RetNet). One of the most representative dominant CORD and COD genes is guanylate cyclase activator A1A (GUCA1A-gene ID: 2978; OMIM: 600364), encoding guanylate cyclase activating protein 1 (GCAP1) . GUCA1A is located at 6p21.1 , and GCAP1 is expressed in the rods and cones as a member of the neuronal calcium sensor family of proteins . This protein is essential for light transduction regulation and confers retinal photoreceptor cells with Ca2+ sensitivity to retGC1 activity [5,6].
Mutations in GCAP1 disrupt calcium binding in GCAP1 or affect GCAP1/retGC1 interaction , thus reducing the Ca2+-dependent inhibition of GCAP1, and leading to increased retGC1 activity and levels of intracellular cyclic guanosine monophosphate (cGMP) [8,9]. Excessive levels of cGMP have been shown to cause retinal degeneration [10,11].
In recent years, 21 mutations in GUCA1A have been identified in patients with vision-threatening retinal diseases [10,12-18], including COD, CORD, macular dystrophy (MD), and central areolar choroidal dystrophy (CACD). Nine missense mutations in GUCA1A have been found in COD (Table 1). This study illustrates a novel missense mutation in GUCA1A (c.431A>G, p.D144G, exon 5) in four generations of a family with adCOD. With functional prediction and analysis, we identified the pathogenic effect of GCAP1-D144G, which can lead to increased retGC1 activity and result in persistently high levels of cGMP. This may also represent a possible mechanism for the formation of adCOD.
Four generations of a family with adCOD were recruited at theQingdao eye hospital of Shandong Eye Institute (Qingdao,China). There were 16 members in the family (7 affected, 9 unaffected; 7 males, 9 females). The 7 affected patients included (I:I, male, 82 years; II:2, female, 63 years; II:3, male, 61 years; III:2, female, 38 years;III:3, male, 37 years; IV:2, female, 8 years; IV:3, male, 15 years).The 9 unaffected patients included (I:2, male, 70years; II:1, male, 65 years; II:4, male, 61 years; III:1, male, 39 years; III:4, male, 37 years; III:5, male, 35 years; III:6, female, 33 years; IV:1, female, 10 years; IV:4, female, 9 years).They all had no other systemic abnormalities. Two hundred individuals with no medical history associated with any ophthalmic diseases were included in the control group. All participants received a comprehensive ophthalmic examination, including measurement of visual acuity and intraocular pressure, color vision testing, fundoscopy, multifocal electroretinography, and optical coherence tomography (OCT). The study was conducted according to the principles of the Declaration of Helsinki and was approved by the Ethics Committee of Qingdao University with informed consent from all participants. Written informed consent were obtained from all participants. The study was conducted according to the principles of the Declaration of Helsinki and ARVO statement for research involving human subjects.
Peripheral venous blood (5 ml) of the participating family members was sampled, and genomic DNA was extracted with a DNA isolation kit for mammalian blood (Tiangen, Beijing, China). Venous blood and genomic DNA samples were stored at −80 °C before useas described . Peripheral venous blood of the participating family members was sampled, and genomic DNA was extracted with a DNA isolation kit for mammalian blood (Tiangen, Beijing, China). The proband (III:2) underwent next-generation sequencing captured with 532 inherited genes related to the genetic visual system. The exon regions of these genes were particularly enriched with a biotinylated capture probe (Joy Orient Translational Medicine Research, Beijing, China). The exon regions of these genes were particularly enriched with a biotinylated capture probe (Joy Orient Translational Medicine Research, Beijing, China)as described . Burrows-Wheeler Aligner (BWA) software was used to perform short-read mapping and alignment, while SOAPsnp software and GATK Indel Genotype were used to test single nucleotide polymorphism (SNP) and insertion and deletion mutations, respectively. Identified mutants were filtered in databases. Sanger sequencing verified whether any remaining variants were cosegregated with the family disease phenotype. The novel mutations in GUCA1A were also genotyped with Sanger sequencing in the 200 normal control subjects. The possible pathogenicity of the mutations was predicted using the Sorting Intolerant from Tolerant (SIFT) algorithm, Polymorphism Phenotyping v2 (PolyPhen-2), Protein Variation Effect Analyzer (PROVEAN), and MutationTaster.
The human GCAP1 protein (NP_000400.2) sequence was aligned for analysis of the conservation of the mutated residues with the sequences of the following orthologous proteins: Bostaurus (NP_776971), Daniorerio (NP_571945), Gallusgallus (NP_989651), Mus musculus (NP_032215), Rattusnorvegicus (NP_001100357), Takifugurubripes (NP_001027790), and Xenopustropicalis (NP_001096291). Multiple alignments were made using ClustalX2 software. The SWISS-MODEL was used to model the homology structure of the GCAP1 mutant based on the chicken wild-type (WT) GCAP1 (Protein Data Bank identifier: 2r2i), and three-dimensional (3D) models of proteins were constructed via PyMol software.
Glutathione-S-transferase (GST)-tagged GCAP1 (GST-GCAP1) was generated via PCR amplification of human GCAP1 cDNA and inserted into pGEX-4T-1. After an initial denaturation step at 94 °C for 3 min, 35 PCRcycles (denaturation: 94 °C, 40 s; annealing: 52 °C, 40 s; extension: 72 °C, 2 min) and a final extension step at 72°C for 10 min were performed. For FLAG-tagging, full-length GCAP1 was inserted into pcDNA3.1. For green fluorescent protein (GFP)-tagging, full-length retGC1 was inserted into the pEGFP-N1 vector to obtain the recombinant plasmid pEGFP-retGC1. GCAP1-D144G was created with PCR amplification and confirmed with sequencing. The methods for expressing fusion proteins were the same as previously described .
Fusion proteins GCAP1-WT and GCAP1-D144G were expressed from the PGEX-4T-1 vector in BL21 (DE3) competent E. coli cells. The overexpressed protein was subsequently purified as described previously  with some modifications. Cells was grown in standard Luria-Bertani (LB) medium (Solarbio, Beijing, China) containing 100 µg/ml ampicillin at 1.0 l, until they reached A600 0.6–0.7. After induction with 0.5 mM isopropyl β-D-thiogalactoside (IPTG) for 2 h, bacterial precipitation obtained with centrifugation at 956 ×g for 30 min at 4 °C was resuspended, and lysozyme was added into the buffer. The cells were then thawed and disrupted with ultrasonication, before 10 mg of streptomycin sulfate was added after the supernatant was centrifuged. The supernatant was centrifuged again, and 60 mg of glutathione agarose (Solarbio, Beijing, China) was added and incubated end-over-end for 2 h at 4 °C. The precipitate was washed with 30 ml of harvest buffer (1 M HEPES, 1 M NaCl, 1 mM benzamidine, and water) after 956 ×g centrifugation at 4 °C. The purity of the final purified GCAP1 protein determined with sodium dodecyl sulfate (SDS) gel electrophoresis was greater than or equal to 95%.
Human embryonic kidney (HEK)-293 cells (Appendix 1) were grown at 37 °C in 5% CO2, incubated, and maintained in complete, high-glucose Dulbecco’s modified Eagle’s medium (HyClone, Logan, UT), which was supplemented with 10% fetal bovine serum and 1% penicillin-streptomycin. According to the manufacturer’s instructions, the cells were transfected with Lipofectamine 2000 (Invitrogen, Carlsbad, CA). During the detection of protein stability, pcDNA3.1-GUCA1A-WT and pcDNA3.1-GUCA1A-D144G were transfected into the HEK-293 cells, and the protein supernatants were extracted for western blotting at 24, 48, and 72 h after transfection. To express retGC1 for the functional assay in vitro, the HEK-293 cells were transiently transfected with a 30 μg of pEGFP-retGC1 plasmid using Lipofectamine 2000 in a 90-mm culture dish according to the manufacturer’s instructions.
Coimmunoprecipitation (co-IP) and western blotting were performed as previously reported . Briefly, HEK-293 cells were transfected with equal amounts of pcDNA3.1-GUCA1A-WT or pcDNA3.1-GUCA1A-D144G in the presence or absence of pEGFP-retGC1, followed by lysis in 1 ml of ice-cold lysis buffer containing 10 mM HEPES, 100 mM NaCl, 1 mM benzamidine, and 0.5% Triton X-100 (pH 7.4). After centrifugation, the lysates were incubated with anti-GFP antibody with protein-A/G agarose (Beyotime Biotechnology, Haimen, China) for 3 h. After being washed with cold wash buffer (10 mM HEPES, 100 mM NaCl, 0.1% Tween-20, benzamidine, and 3% bovine serum albumin [BSA]) three times, the immunoprecipitated proteins were eluted from the beads with SDS sample loading buffer. The co-IP assay was performed using anti-GFP affinity gel, while the bound proteins were detected with immunoblotting with anti-FLAG antibody. Then, the eluted samples were separated with SDS–polyacrylamide gel electrophoresis (PAGE), visualized with western blotting, and quantified by NIH Image 1.62. Each sample was normalized with glyceraldehyde-3-phosphate dehydrogenase (GAPDH). Primary antibodies included anti-FLAG antibody (Proteintech Group, Chicago, IL), anti-GFP antibody (Proteintech Group), and anti-GAPDH antibody (Kangchen, Shanghai, China).
Limited protein hydrolysis of purified GCAP1 and GCAP1-D144G was observed in SDS–PAGE in the presence or absence of 2.5 μM Ca2+ as previously described . Purified recombinant GCAP1 or GCAP1-D144G was incubated with trypsin at 30 °C, and the digest was analyzed with SDS-PAGE at 0, 5, 10, and 20 min.
The HEK-293 cells were cotransfected with pEGFP-retGC1 and pcDNA3.1-GUCA1A-WT/D144G plasmid as previously reported. The following is a supplement to the protocol’sdetails. PEGFP-retGC1 and pcDNA3.1-GUCA1A-WT / D144G plasmids were co-transfected into HEK-293 cells with a GCAP1: retGC1 plasmid ratio of 1: 0.5. According to the reagent manufacturer's instructions, the cells were transfected with Lipofectamine 2000 The slides of the cells cultured in the standard glass coverslip chambers (four 2 cm2 chambers per slide) were washed twice with PBS (1X; 8 mM Na2HPO4, 137 mM NaCl, 2mM KH2PO4, 2.6 mM, KCL, pH 7.2), fixed with 4% paraformaldehyde for 15 min, and washed again following permeation with 0.2% Triton X-100. After being blocked overnight with 5% normal goat serum, the samples were incubated with anti-FLAG antibody at 37 °C for 1 h, washed, and stained with a fluorescein-conjugated second antibody (donkey anti-rabbit immunoglobulin (IgG; H+L; Life Technologies, Carlsbad, CA) at 37 °C for 30 min. The cell nucleus was counterstained with 4’, 6-diamidino-2-phenylindole (DAPI) for 5 min and then washed as mentioned above. Cells were observed using a fluorescence microscope (CKX53, Olympus, Tokyo, Japan).
pcDNA3.1-GUCA1A-WT and pcDNA3.1-GUCA1A-D144G were transfected into the HEK-293 cells. The cell pellets were divided into groups of EGTA (1 μM EGTA) and Ca2+ (2.5 μM Ca2+) after they were homogenized in 300 µl of lysis buffer with the added protease inhibitor cocktail.
Human retGC1 was expressed in the HEK-293 cells, and the washed cell membranes were prepared as previously described . HEK-293 cells were transiently transfected with pEGFP-retGC1 plasmid using Lipofectamine 2000 according to the manufacturer and purification of membrane fractions containing expressed cyclase as previously described . Briefly, the membranes containing equal amounts of total protein were resuspended in GC buffer (100 mM KCl, 50 mM Mops, 7 mM 2-mercaptoethanol, 8 mM NaCl, 10 mM MgCl2, 1 mM EGTA). Cell membranes were incubated with equal amounts of purified GCAP1-WT/D144G proteins, and the cGMP concentrations were measured at different free Ca2+ levels using a Ca2+-EGTA buffer system (1 μM EGTA or 2.5 μM Ca2+).
Protein concentrations were standardized by extracting the protein and using a bicinchoninic acid (BCA) protein assay kit. Human cGMP competition enzyme-linked immunosorbent assay (ELISA; human cGMP ELISA Kit; Mlbio, Shanghai, China) was used to determine the cGMP levels following the manufacturer’s instructions.
SPSS 19.0 was used for statistical analysis, and quantitative data were analyzed by using the Student t test to compare groups. The data are presented as the mean ± standard deviation (SD), and a p value of less than 0.05 was considered statistically significant.
Ophthalmic examination confirmed that seven of 16 members across the four generations of the sampled family were affected by adCOD (Figure 1). All patients had similar features, including progressive vision loss, photophobia, nystagmus, color vision impairment, and visual field impairment. The proband (III:2) was a female patient aged 43 years at the time of observation. Her best corrected visual acuity was oculus dexter (OD) 0.1 and oculus sinister (OS) 0.05. The fundus appearance (Figure 2A,B) and macular OCT (Figure 2C) were consistent with the diagnosis. Patient IV:3 was first seen at age 16. His best corrected visual acuity was OD 0.5 and OS 0.4. His fundoscopy (Figure 3A,B) and macular OCT (Figure 3C) results were also in accordance with the diagnosis. For IV:3, the multifocal electroretinography examination showed that the amplitude density of the left eye’s macular area was significantly reduced (Figure 3D). Humphrey visual field examination showed that the visual fields of both eyes were defected to different degrees (Figure 3E).
The proband (III:2) was genetically tested with exome sequencing of a set of candidate genes. The average sequence depth was 58.34, and 72.21% of the exon sequences were sequenced at least ten times. Sixty-two non-synonymous SNPs, two splicing sites, and one indel were selected according to the recommended filtering criteria. In exon 5 of GUCA1A, only a novel missense mutation (c.431A > G, p.D144G) was cosegregated in the family (Figure 4A and Table 1). This mutation was not found in the 200 control individuals. PolyPhen-2 and SIFT predicted that the D144G missense mutation would lead to harmful changes in the function of GUCA1A (Table 1).
D144 located in the EF4 hand loop was involved in calcium binding (Figure 4B,C). Multiple alignments of D144 of the GCAP1 protein from different species revealed 100% identification, which suggested it was highly conserved during evolution (Figure 4B). The homology structure of GCAP1-D144G (Figure 4C) showed that the hydrogen bonds between residue 144 and residue Phe140 or Gly147 in GCAP1 were eliminated due to substitution from Aspartyl (Asp) to Glycine (Gly) (Figure 4D).
We assayed the ability of GCAP1-WT and GCAP1-D144G to regulate retGC1in vitro (Figure 5A). The concentration of cGMP in the Ca2+ group became lower than that in the EGTA group after induction by GCAP1-WT (p<0.05), whereas it was higher than that in the EGTA group due to induction by GCAP1-D144G (p<0.01). GCAP1-D144G caused a statistically significant increase in the cGMP concentration compared to GCAP1-WT (p<0.01) in the presence of Ca2+. The same experimental result was also found in vitro (Figure 5B). GCAP1-D144G led to a higher increase of cGMP synthesis than did GCAP1-WT (p<0.01; Figure 5B).
To detect the effect of GCAP1-D144G on the protein structure, limited protein hydrolysis experiments were performed. In the absence of Ca2+, GCAP1-WT was readily susceptible to proteolysis after 5 min of exposure to trypsin, while GCAP1-D144G was completely digested (Figure 6A), indicating the open conformation of GCAP1-WT and D144G. Furthermore, the tight core of GCAP1-WT remained after 20 min of digestion in the presence of Ca2+. Under the same condition, GCAP1-D144G was more susceptible to hydrolysis after 20 min of exposure to trypsin (Figure 6A). It indicated that GCAP1-WT exhibited a tighter conformation than D144G in the presence of Ca2+.
The electrophoresis shift assay showed that GCAP1-WT exhibited a higher degree of electrophoretic mobility than GCAP1-D144G in the presence of Ca2+ (Figure 6B), which was typical for calmodulin-like Ca2+ binding proteins (the faster-moving, inactive form). However, the same experiment with GCAP1-D144G highlighted slower mobility during the electrophoresis shift assay in the presence of Ca2+, indicating that the Ca2+ induction of the mutant conformation was less pronounced, indicating a significantly decreased affinity for Ca2+.
The expression levels and stability of GCAP1 in HEK-293 cells were analyzed with western blotting. With the extension of the transfection time, the GCAP1-WT protein levels remained almost unchanged (Figure 6C). However, the levels of GCAP1-D144G decreased statistically significantly in a time-dependent manner (Figure 6C). Even after 72 h of transfection, the expression levels of GCAP1-D144G were statistically significantly lower than those of GCAP1-WT (p<0.01; Figure 6C).
To determine whether GCAP1-WT/D144G was colocalized with retGC1, the HEK-293 cells were cotransfected with FLAG-GCAP1-WT/D144G and GFP-retGC1. GCAP1-WT and GCAP1-D144G exhibited a similar membrane distribution, predominantly endoplasmic reticulum membranes, when they were coexpressed with retGC1 (Figure 7A).
To test the ability of GCAP1-WT/D144G to bind to retGC1, co-IP experiments were performed. As shown in Figure 7B, the FLAG-GCAP1 protein was not detectable in the immunoprecipitated complex in the cells transfected with FLAG-GCAP1-WT or FLAG-GCAP1-D144G alone. In the cells cotransfected with FLAG-GCAP1 and GFP-retGC1, however, the FLAG-GCAP1 protein could be detected in its immunoprecipitated complex. GCAP1-D144G enhanced the association of GCAP1 with retGC1 in HEK-293 cells.
Mutations in GUCA1A have been found in CORD, which is a blinding eye disease affecting 1/30,000 to 1/40,000 individuals . Some common features of retinal dystrophies associated with these mutations have been identified [10,12-14]. However, the molecular characteristics do not necessarily relate to similar clinical phenotypes . Therefore, the molecular mechanism and function of each mutation must be investigated.
GCAP1 contains four EF hand motifs (EF1–4), with each containing a helix–loop–helix conformation . EF1 and EF2 form the N-terminal domain, whereas EF3 and EF4 are contained in the C-terminal region . EF1 is modified for the interface with guanylate cyclases (GCs) , while EF2, EF3, and EF4 bind to Ca2+ . Among the 21 previously reported mutations in GUCA1A, two were deletion mutations, and the others were missense mutations, including nine missense mutations found in patients with COD. This study recruited four generations of a family with adCOD exhibiting clinical phenotypes of adCOD, such as progressive vision loss, abnormalities of color vision, and nystagmus. Genetic tests detected a novel mutation in GUCA1A (c.431A>G, p.D144G, exon 5) in the family. The characteristics of the clinical phenotypes, their molecular features, and specific functions of the mutant protein were subsequently evaluated.
Biochemically, most mutations in GCAP1 are located in the EF hand regions. Ile143AsnThr , Leu151Phe [27-29], Glu155Gly , and Gly159Val , which are located in EF4, disrupt calcium binding in GCAP1 or affect GCAP1/retGC1 interactions . Thus, reducing Ca2+-dependent inhibition of GCAP1 could promote the constitutive activity of retGC1 and increase the intracellular cGMP levels [8,9,32], ultimately leading to photoreceptor death. The novel missense mutation (p.D144G) found in this research was also located in EF4. Biochemical results disclosed that the substitution of ASP with 144 GLY may partially impair GC1 inhibition, which constitutively activated retGC1 at the normal, dark Ca2+ levels and generated a continuous increase in the intracellular cGMP levels. The calcium sensitivity effect of mutations in reducing GC stimulation has also been seen in Y99C , N104K , E111V , T114I , 143NT , L151F [27-29], and E155G .
Sequence analysis showed that the 144 ASP was highly conserved. It was necessary for the correct coordination of Ca2+ in the EF4 loop with high affinity sites. The SWISS-MODEL was used to model the homology structure of GCAP1-D144G on the basis of GCAP1. It was shown that the hydrogen bonds between residue 144 and residue PHE140 or GLY147 in GCAP1-WT were eliminated due to the substitution of ASP with 144 GLY. These hydrogen bonds appeared to be important for the tertiary structure of the protein because they linked the EF3 helix and the EF4 loop. Therefore, GCAP1-D144G may result in the loss of hydrogen bonds in the protein, interfering with correct GCAP1 folding.
Limited protein hydrolysis experiments indicated that GCAP1-D144G was more susceptible to proteolysis. GCAP1-D144G cannot presume a compact Ca2+-bound conformation, which was necessary for the inactivity in dark Ca2+. The same effects have been observed in GCAP1-N104K , L151F [27,28], and I143NT . GCAP1-N104K, located in the EF3 loop, was replaced by positive-charge amino acids and destroyed the binding of the EF3 hand to Ca2+ . GCAP1-L151F was in the β-folding of the EF4 hand, and its molecular dynamic confirmed that changes in the mutant structure affected the binding of Ca2+ in the EF4 and EF2 hands . GCAP1-I143NT was located on the EF4 hand helix. The substitution of Ile143 with two polar residues changed the orientation of the N-terminal α-helix, which reduced the affinity of the EF hands to Ca2+ .
An electrophoretic shift assay showed that Ca2+ binding resulted in lower electrophoretic mobility of GCAP1-D144G in the presence of 2.5 μM Ca2+ while GCAP1-WT showed higher mobility. This suggested that the affinity of the mutant for Ca2+ was significantly reduced. With respect to the protein stability, the expression levels of GCAP1-D144G significantly decreased as the transfection time was prolonged. The expression levels of the WT protein were almost identical, indicating a decrease in the stability of the mutant protein. Similarly, GCAP1-P50L showed decreased thermal stability . These biochemical results illustrated that the GCAP1-D144G mutation could prevent proteins from folding into compact structures.
GCAP1 and retGC1 may control the recovery of light response in the photoreceptors of vertebrates through their molecular interactions and retGC1 in rods involved in regulating cGMP synthesis by negative calcium feedback . Studies have shown that mutations in GCAP1 or retGC1 could alter the Ca2+ sensitivity of cGMP synthesis or affect the GCAP1/retGC1 interaction [7,8,22,30,36,37]. Therefore, even at higher calcium concentrations, mutations in GCAP1 can stimulate retGC1 , and ultimately, lead to degeneration and death of photoreceptors [10,11,13]. However, the mechanism by which mutations affect the GCAP1/retGC1 interaction is complex and difficult to understand . GCAP1 activation of retGC1 may be performed either by direct binding or by indirect interaction . Indirect interaction is consistent with the experimental results of previous studies on the binding of Ca2+- and Mg2+-saturated forms of retGC1 [40-42]. The conversion from activator to inhibitor status by Ca2+ bound to EF4 in GCAP1 is a major determinant .
It was found that GCAP1-D144G not only displayed colocalization with retGC1 in the HEK-293 cells (Figure 7A) but also combined more retGC1 in the HEK-293 cells (Figure 7B). However, mutations in different parts of GCAP1 disrupted the colocalization of GCAP1/retGC1, allowing most of the GCAP1 fluorescence to be evenly distributed across the cytoplasm and nucleoplasm . We observed only the changes in colocalization caused by the mutation. The specific mechanism must be further explored. In addition, metal ligand binding in EF4 has been reported to have no significant effect on GCAP1 association with the cyclase . The areas of GCAP controlling its ability to activate retGC1 are the interface between EF1, EF2, EF3, and the adjacent C-terminal region of EF4 [45,46]. EF1 has evolved in GCAPs to become the main part of the target-binding interface [39,40]. Moreover, EF2 and EF3 can be connected to retGC1 through the combination of Ca2+ or Mg2+ . Therefore, it is suspected that the binding of GCAP1-D144G to retGC1 may strongly affect the indirect interaction or that the structure of EF1 can be remotely affected by Ca2+ binding on the EF4 hand.
The process and mechanism of the interaction between GCAP1 and retGC1 after point mutation, as well as the changes in key residues and conformations involved, require further investigation. Based on the genetic testing and functional analyses, we concluded that the novel GCAP1-D144G mutation affected Ca2+ sensitivity and the constitutive activation of retGC1 at high Ca2+ levels, resulting in increased intracellular cGMP concentrations, and ultimately, likely adCOD. These findings help to introduce the diversity of phenotypes, providing guidance for clinical assessment and treatment of adCOD.
Appendix 1. STR analysis.
The authors thank all patients and their family for participating in the study. This work was supported by the National Natural Science Foundation of China (No. 81,970,782, No. 81,600,721), Shandong Provincial Natural Science Foundation (No. ZR2018MH016), Qingdao Postdoctoral Application Research Project (No. 40,518,060,071), China Postdoctoral Science Foundation (No. 2017M612211), Medical and Health Technology Development Project of Shandong Province (No. 2016WS0265), and Higher Educational Science and Technology Program of Shandong Province (No. J17KA235). Dr. Peng Chen (firstname.lastname@example.org) and Dr. Xiaojing Pan (email@example.com) are co-corresponding authors for this study.