Article Text

Original research
GLRA2 gene mutations cause high myopia in humans and mice
  1. Qi Tian1,2,3,
  2. Ping Tong4,
  3. Gong Chen2,3,5,6,
  4. Meichun Deng2,3,5,6,
  5. Tian'e Cai7,
  6. Runyi Tian1,2,3,
  7. Zimin Zhang1,2,3,
  8. Kun Xia1,2,3,
  9. Zhengmao Hu1,2,3
  1. 1Center for Medical Genetics, School of Life Sciences, Central South University, Changsha, Hunan, People's Republic of China
  2. 2Hunan Key Laboratory of Medical Genetics, School of Life Sciences, Central South University, Changsha, Hunan, People's Republic of China
  3. 3Hunan Key Laboratory of Animal Models for Human Disease, School of Life Sciences, Central South University, Changsha, Hunan, People's Republic of China
  4. 4Department of Ophthalmology, The Second Xiangya Hospital, Central South University, Changsha, Hunan, People's Republic of China
  5. 5Hunan Province Key Laboratory of Basic and Applied Hematology, School of Life Sciences, Central South University, Changsha, Hunan, People's Republic of China
  6. 6Department of Biochemistry and Molecular Biology, School of Life Sciences, Central South University, Changsha, Hunan, People's Republic of China
  7. 7Reproductive Center, Sanya Central Hospital, Sanya, Hainan, People's Republic of China
  1. Correspondence to Professor Zhengmao Hu, Center for Medical Genetics, School of Life Sciences, Central South University, Changsha, Hunan, People's Republic of China; huzhengmao{at}sklmg.edu.cn; Dr Ping Tong, Department of Ophthalmology, The Second Xiangya Hospital, Central South University, Changsha, Hunan, People's Republic of China; tongping{at}csu.edu.cn; Professor Kun Xia, Center for Medical Genetics, School of Life Sciences, Central South University, Changsha, Hunan, People's Republic of China; xiakun{at}sklmg.edu.cn

Abstract

Background High myopia (HM) is a leading cause of blindness that has a strong genetic predisposition. However, its genetic and pathogenic mechanisms remain largely unknown. Thus, this study aims to determine the genetic profile of individuals from two large Chinese families with HM and 200 patients with familial/sporadic HM. We also explored the pathogenic mechanism of HM using HEK293 cells and a mouse model.

Methods The participants underwent genome-wide linkage analysis and exome sequencing. Visual acuity, electroretinogram response, refractive error, optical parameters and retinal rod cell genesis were measured in knockout mice. Immunofluorescent staining, biotin-labelled membrane protein isolation and electrophysiological characterisation were conducted in cells transfected with overexpression plasmids.

Results A novel HM locus on Xp22.2-p11.4 was identified. Variant c.539C>T (p.Pro180Leu) in GLRA2 gene was co-segregated with HM in the two families. Another variant, c.458G>A (p.Arg153Gln), was identified in a sporadic sample. The Glra2 knockout mice showed myopia-related phenotypes, decreased electroretinogram responses and impaired retinal rod cell genesis. Variants c.458G>A and c.539C>T altered the localisation of GlyRα2 on the cell membrane and decreased agonist sensitivity.

Conclusion GLRA2 was identified as a novel HM-causing gene. Its variants would cause HM through altered visual experience by impairing photoperception and visual transmission.

  • genetics, medical
  • human genetics
  • eye diseases
  • ophthalmology
  • genetic variation

Data availability statement

All data relevant to the study are included in the article or uploaded as supplementary information. Not applicable.

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This is an open access article distributed in accordance with the Creative Commons Attribution Non Commercial (CC BY-NC 4.0) license, which permits others to distribute, remix, adapt, build upon this work non-commercially, and license their derivative works on different terms, provided the original work is properly cited, appropriate credit is given, any changes made indicated, and the use is non-commercial. See: http://creativecommons.org/licenses/by-nc/4.0/.

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Key messages

What is already known on this topic

  • High myopia is one of the leading causes of blindness with high global prevalence; however, the genetic and pathogenic basis of high myopia remains largely unknown.

What this study adds

  • This study identifies a novel high myopia causal gene, GLRA2, encoding the glycine-gated chloride channel subunit GlyRα2.

  • Mouse-model study reveals that GlyRα2 plays a role in vision transmission and rod cell genesis in vivo.

How this study might affect research, practice and/or policy

  • This study provides confidential evidence for the conception that abnormal visual experience is a driver for high myopia and chloride channel is involved, further benefiting the genetic counselling, precise intervention and control of high myopia progression.

Introduction

Refractive error (RE) is the leading cause of moderate and severe visual impairment and the seventh most prevalent clinical condition globally.1–3 Four common types of RE are hyperopia, myopia, astigmatism and presbyopia, but myopia is the dominant RE form.2 3 Currently, there is no internationally agreed quantitative threshold for HM. WHO indicates the threshold for HM of RE ≤−5.00 diopters (D),4 and the International Myopia Institute (IMI) define the HM as RE below −6.00 D when ocular accommodation is relaxed.5 HM is a progressive disorder that begins in early childhood and worsens overtime, even after adulthood.6 HM can be accompanied by elongated axial length, lacquer cracks, retinal atrophy, macular holes and neovascularisation, etc, and it is one of the leading causes of blindness.7 Myopia and HM rates are predicted to reach 49.8% and 9.8%, respectively, worldwide by 2050.8 According to the twin study, the hereditary of myopia varies from 50% to 90%.9 10 To date, next-generation sequencing and genome-wide linkage analysis have identified 25 HM loci, and 16 causal genes.11 12 Moreover, genome-wide association studies and other association studies have uncovered approximately 200 myopia-associated loci. However, these genetic factors can explain only a minority of HM cases, despite its high prevalence in humans.13

The eye is an elastic organ that is enveloped by an extracellular matrix (ECM)-rich structure called sclera and looks like a ball in the presence of intraocular pressure (IOP).14 Abnormal development of the eye and ECM are the two widely accepted factors causing HM.15–18 On the one hand, the genetic or environmental effectors cause uncontrolled eye enlargement during early development, ultimately leading to HM after birth.17–19 On the other hand, the intrinsic and extrinsic factors that cause abnormal ECM synthesis and catalysis increase the elasticity and decrease the tension of the sclera.16 Under these conditions, IOP enlarges the eye resulting in HM.11 16 18 However, these mechanisms cannot explain the large number of patients with HM. Recently, increasing evidence has emerged to support the idea that HM can be a visually driven abnormality.20 21 Genetics studies have shown that many HM-related genes, such as OPN1LW,22 RDH512 and NYX,23 are associated with photopic perception, retinal circuit and visual transmission. These findings indicate that impaired visual experience, mainly composed of photoperception and visual information transmission, may play a vital role in HM onset and development.12 15 20 Emmetropisation is a vision-dependent process that controls the development of RE and eye growth.24 Gene mutations that cause impaired visual experience may result in overemmetropisation and uncontrolled eyeball growth, thereby leading to HM.12 25

Thus, we aimed to explore the genetic mechanisms of HM by studying 38 individuals (composed of 18 patients and 20 normal subjects) from two unrelated Chinese families with HM and 200 patients with familial/sporadic HM. Using genome-wide linkage analysis combined with exome sequencing (ES) and Sanger sequencing screening, we identified two HM-related variants in GLRA2 gene (GenBank: NM_002063.4, NP_002054.1): c.458G>A (p.Arg153Gln) and c.539C>T (p.Pro180Leu). Moreover, we constructed knockout mice using the CRISPR/Cas9 system and analysed their myopic phenotypes, retinal morphology and rod cell differentiation to elucidate the mechanism of HM pathogenesis.

Methods

Subjects and clinical examination

This study recruited individuals from two unrelated families with HM (HM1 and HM2) and 200 patients with familial/sporadic HM from the Chinese population. HM1 and HM2 families included 8 and 10 patients with HM, respectively, and 10 asymptomatic subjects each family. Among the 200 patients with familial/sporadic HM recruited, the gender ratio was 79:121 (male:female). In adult subjects, HM was defined using the WHO recommended threshold as RE ≤−5.00 D in either eye.5 Subjects younger than 15 years with moderate myopia (−3.00 D≤RE˂−5.00 D) were also considered as patients with HM.

All ophthalmological examinations were performed at the Second Xiangya Hospital, Central South University. Visual acuity and refraction were measured using a LogMAR chart and autorefractor (Huvitz HRK-1 Autorefractor, Coburn Technologies, Singapore), respectively. The lens and vitreous were measured using a slit lamp (Huvitz Slit Lamp HS-5000, Coburn Technologies, Singapore), retina using an ophthalmoscope (NTZ-OPH-BXa-RC Neitz Ophthalmoscope, Neitz Instruments, Japan) and axial length using an A-scan ultrasound device (ABSolu A/B/S/UBM Ultrasound Platform, Quantel Medical, France).

Genome-wide linkage analysis and haplotyping

Eighteen samples from the HM1 family were genotyped using Illumina iScan system (Illumina, USA) and Illumina HumanCytoSNP-12 V.2.1 BeadChip kit. Genotypes were called and quality controlled using Illumina GenomeStudio 2011. Genome-wide linkage disequilibrium of HM1 family was tested by merlin V.1.1.226 under multiple-parameter analysis with ‘High_myopia 0.001 0.001,0.9,0.99 rare_dominant’ settings. The ‘merlin’ or ‘minx’ prompt was used to analyse the autosomal or X linked linkage disequilibrium separately. Merlin V.1.1.2 drew the haplotype of HM1 and HM2 families with the ‘best’ option.

Exome sequencing

The gDNA of HM1-I:2, HM1-II:4, HM1-III:10, HM2-III:4, HM2-IV:5 and HM2-IV:6 were analysed through ES as previously described.27 Briefly, the library was captured using Agilent SureSelectXT Human All Exon V4+UTRs probe and sequenced on Illumina HiSeq 2000 sequencing system (Illumina) with PE100. The reads were then aligned to the human genome assembly GRCh37/hg19 using bwa 0.7.10.28 Variants were called with GATK 3.2.229 and annotated using ANNOVAR.30

After screening out variants with allele frequency >0.01 in the gnomAD (https://gnomad.broadinstitute.org/) and 1000 Genomes Project (https://www.internationalgenome.org/) databases, all patients shared non-synonymous variants (including single nucleotide variants (SNVs) and insertion-deletion polymorphisms (indels)) in the consensus coding sequence (CCDS), and the canonical splicing sites were reserved. Variants within the linkage region were selected for co-segregation analysis.

Primer design and co-segregation analysis of the candidate variants

All primers were designed using the online software Primer3 (https://primer3.ut.ee/) based on the human GRCh37/hg19 or mouse GRCm38/mm10 assemblies (online supplemental table 1). PCR and Sanger sequencing were performed to confirm the co-segregation status of the candidate variants in the samples of HM families and to screen for gene variants in the samples of patients with familial/sporadic HM.

Visual acuity and refractive error evaluation of Glra2 knockout mice

Glra2 knockout mice were developed by zygote injection of CRISPR/Cas9 mRNA and a pair of gRNAs flanking the second exon of Glra2 gene (GenBank: NM_183427.5), which was shared by all isoforms. It was predicted that the deletion of this exon would cause a frameshift during Glra2 mRNA translation. Knockout efficiency was validated using RT-PCR and Sanger sequencing of the mRNA extracted from the retina of adult knockout mice. All the animals evaluated were male. Visual acuity was assessed under 100 lux light intensity following the protocol by Prusky et al.31 RE was measured using an eccentric infrared photorefractor (custom built) according to the method by Schaeffel et al.32

Ocular biometry measuring and electroretinography recording

The ocular biometry of Glra2 knockout mice, including corneal radius, corneal thickness, chamber depth, lens thickness, vitreous depth, retinal thickness and axial length, was measured using optical coherence tomography (OCT) following the protocol by Zhou (custom built).33 Electroretinography (ERG) recording was performed using a six-step workflow following the modified instructions of the International Society for Clinical Electrophysiology of Vision. Briefly, mice were dark-adapted for at least 4 hours and anaesthetised by the intraperitoneal administration of ketamine and xylazine mixture. The pupils were then dilated with compound tropicamide eye drops and the electrodes were placed at their corresponding positions. Dark-adapted scotopic 0.01, scotopic 3.0, scotopic 10.0 and oscillatory potentials (OPs) were recorded sequentially using a RETI-port/scan 21 system (Q450SCX, Roland Consult, Germany). After 2 min of light adaptation, photopic 3.0 and photopic 3.0 flicker 30 Hz responses were recorded.

Immunohistofluorescence and H&E staining of mouse retina

Paraffin-embedded mice eyeballs were sagittally sectioned into 4 µm slices using paraffin microtome (RM2235, Leica Biosystems, Germany). Paraffin sections were dewaxed and rehydrated and permeated with 0.1% Triton-X in 1× phosphate-buffered saline (PBS) at room temperature. The sections were then blocked with 5% bovine serum albumin (BSA) in 1× PBS containing 0.3M glycine and incubated overnight with a primary antibody diluted with 5% BSA in 1× PBS at 4°C. After incubation with a fluorescent-conjugated second antibody and the nuclear staining with 4′,6-Diamidino-2-phenylindole dihydrochloride (DAPI), the sections were mounted and captured using a confocal microscope (Leica TCS SP5, Leica Biosystems). The primary antibody used was anti-rhodopsin (Cat: ab98887, Abcam, USA).

OCT-embedded eyeballs were sagittally sectioned into 14 µm slices using a cryostat microtome (CM1850, Leica Biosystems). OCT-embedded sections were postfixed with 4% paraformaldehyde (PFA) and stained using an H&E staining kit according to the manufacturer’s instructions (Cat: ab245880, Abcam).

Cell culture and immunofluorescent staining

HEK293 cell line (American Type Culture Collection) was cultured in high-glucose Dulbecco’s Modified Eagle Medium containing 10% fetal bovine serum (FBS) and transfected with wild-type (WT), GLRA2R153Q, GLRA2P180L and GLRA2V341I overexpression plasmids using Lipofectamine 2000 reagent (Cat: 11668030, Thermo Scientific, USA).

The retina of P5.5 age mice were dissected and dissociated using papain and DNase I. The resuspended cells were cultured in a Lab-Tek Chamber with minimum essential medium containing 10% FBS.

The HEK293 and retina cells were washed with 1× PBS, fixed with 4% PFA, and then permeated with 0.1% Triton-X in 1× PBS or non-permeated with 1× PBS at room temperature. The cells were stained with the same procedures used for immunohistofluorescence (IHF) staining. The primary antibodies used were anti-GlyRα2 (Cat: ab97628, Abcam) and anti-rhodopsin (Cat: ab98887, Abcam).

Detection of biotin-labelled membrane proteins of transfected HEK293 cells

Membrane proteins were biotinylated following the manual instructions of the EZ-Link Sulfo-NHS-LC-Biotinylation kit (Cat: 21435, Thermo Scientific). For western blot analysis detection, the samples were separated on a 12% sodium dodecyl sulfate-polyacrylamide gel electrophoresis and transferred to a polyvinylidene fluoride membrane. The membranes were incubated with a primary antibody overnight at 4°C. The primary antibodies used were anti-GlyRα2 (Cat: ab97628, Abcam), anti-E-cadherin (Cat: ab15148, Abcam) and anti-GAPDH (Cat: ab9484, Abcam). Next, the horseradish peroxidase-conjugated secondary antibody was incubated for 1 hour at room temperature, and the bands were visualised using the ECL substrate.

Electrophysiology experiment

After HEK293 cells were transfected with overexpression plasmids, the whole-cell currents were recorded using the HEKA EPC9 system (Harvard Bioscience, USA) under voltage-clamp mode at −60 mV at 25°C±1°C. The patch-pipette resistance was approximately 1–3 MΩ when filled with intracellular buffer, and the glycine solutions (0.01 mM to 1 M) were applied by the ‘U’ tube incubation system. Extracellular buffer: NaCl 140.0 mM, KCl 5.0 mM, CaCl2 2.0 mM, MgCl2 1.0 mM, N-2-hydroxyethylpiperazine-N-ethane-sulphonicacid (HEPES) 10.0 mM, D-glucose 10.0 mM; pH adjusted to 7.4 with NaOH. Intracellular buffer: CsCl 145.0 mM, MgATP 2.0 mM, CaCl2 2.0 mM, MgCl2 2.0 mM, ethylene glycol tetraacetic acid 10.0 mM, HEPES 10.0 mM; pH adjusted to 7.4 with caesium hydroxide. Normalised concentration-response curves were fitted using the following equation:

Embedded Image

where I/Imax is the normalised current amplitude, EC50 is the glycine concentration that evokes half of the maximal response and H is the Hill coefficient.

Statistics analysis

The statistical significance of the differences in the OPs, photopic a and b wave, photopic 3.0 flicker 30Hz amplitude, normalised ocular parameters, retinal layer thickness, visual acuity, and RE between Glra2 knockout and WT mice was determined using paired t-test with a two-tailed p-value. A two-way analysis of variance was used to assess the difference in dark-adapted ERG a-wave and b-wave amplitude between Glra2 knockout and WT mice. The dose-normalised response was non-linearly regressed using a variable slope. Statistical significance was set at p≤0.05.

Results

Clinical characteristics

In HM1 family, patients with HM (figure 1A and table 1) presented eye RE ranging from −15.00 to −5.50 D. Fundus photography revealed that patients II:2, II:4, III:5 and IV:4 with bilateral tigroid fundus; patients I:2, II:4 and IV:4 with retinal atrophy (figure 2). Moreover, patient III:11 presented a decreased dark-adapted ERG response to the scotopic 0.01 b, scotopic 3.0 a and b and OP waves (figure 2A,B). In HM2 family, patients with HM (figure 1A and table 2) presented eye RE ranging from −11.00 to −3.25 D. Among the 200 patients with familial/sporadic HM recruited, eye RE ranged from −33.00 to −5.50 D.

Figure 1

Genetic studies of high myopia (HM) families and sporadic patients. (A) Pedigree of two HM families and Sanger sequencing of c.458G>A (p.Arg153Gln) and c.539C>T (p.Pro180Leu) variants in GLRA2 gene. (B) Genome-wide multipoint linkage analysis of HM1 family. (C) Schematic structure of GlyRα2 and three missense variant’s locations. (D) Amino acid conservation alignment of Arg153, Pro180 and Val341. The arrow in the pedigree indicates the proband. ‘□’ and ‘○’ symbols present asymptomatic male and female subjects, respectively; ‘■’ and ‘●’ characters stand for male and female patients, respectively. Samples selected for exome sequencing (ES) were marked with ‘*’. ‘+’ stands for wild-type allele and ‘-’ refers to c.539C>T allele.

Table 1

Clinical characteristics in HM1 family

Table 2

Clinical characteristics in HM2 family and sporadic HM patient M21227

Figure 2

Clinical features of patients in HM1 family. (A) Dark-adapted electroretinography results of asymptomatic subject III:14 and patient III:11. (B) Fundus of asymptomatic subject III:9, female patient II:4 and male patient IV:4. HM, high myopia; OP, oscillatory potential.

c.539C>T (p.Pro180Leu) variant in GLRA2 gene co-segregated with high myopia

In HM1 family, all subjects participated in linkage analysis. As IV:4 was highly myopic, we proposed his mother III:9 should be an obligate carrier. Parametric multipoint linkage analysis of HM1 family showed no known HM locus throughout the genome. On auto-chromosome, two regions, 5q33.3-q34 and 8q21.12-q24.13, with a maximum logarithm of odds (LOD) score of only 1.008 and 1.39, respectively were identified. In addition, we identified a novel highly linked locus of approximately 24.7 Mb on Xp22.2-p11.4, with a maximum LOD score of 2.88, surrounding the marker rs4825340 (figure 1B and online supplemental table 2). No known HM causal genes were found in this linkage region.

Through ES of patients I:2, II:4 and III:10 from HM1 family, we harvested 12.6, 11.4 and 11.3 Gb raw data with mean depth of 128, 118 and 121, respectively. We identified 35 483 combined variants (including SNVs and indels) with a frequency below 0.5 in the 1000 Genomes Project by annotation. Finally, we got 1192 shared non-synonymous variants within the CCDS and canonical splicing sites with a frequency lower than 0.01 in the gnomAD_Genome_asn, gnomAD_ExAc_asn and maf1000g_asn databases. No mutations were identified in the known HM-causing genes.

Genome-wide linkage analysis, ES and Sanger sequencing revealed that only the rare non-synonymous variant in the linkage loci, GLRA2: c.539C>T (p.Pro180Leu), was co-segregated with the HM phenotype in HM1 family, and that III:9 was heterozygote (figure 1A). ES and Sanger sequencing data indicate that the c.539C>T variant was also co-segregated with HM phenotype in HM2 family (figure 1A and table 2). Moreover, II:2 was a heterozygote and had normal vision. The haplotypes of the ES samples with the c.539C>T variant were then included to determine whether the variant was located on the same haplotype in both families. We found that HM1 and HM2 families had different haplotypes from rs3764879 through c.539C>T to rs2229137, suggesting no founder effect (online supplemental figure 1A).

Two additional rare variants were identified by screening GLRA2 gene in the 200 unrelated patients with familial/sporadic HM: c.458G>A (p.Arg153Gln) in sporadic sample M21227 and c.1021G>A (p.Val341Ile) in IV:1 from HM3 family. Sanger sequencing results showed that c.1021G>A variant descended from II:3 and III:2 which were emmetropic. Variant c.1021G>A did not co-segregated with HM phenotype in HM3 family (online supplemental figure 1B). Therefore, variant c.1021G>A may be a polymorphism.

Glra2 knockout mice had myopic phenotypes

To further confirm the relationship between GLRA2 gene and HM, a Glra2 knockout mouse model was used. Detailed inspection revealed that Glra2 knockout mice had regular overall postnatal developments and that each individual was born at a Mendelian ratio without morphological abnormalities. Glra2 knockout mice also behaved normally, so did their WT littermates.

We evaluated the visual acuity of Glra2 knockout mice with a modified Y-maze according to the methods by Prusky et al.31 After two training days, all mice passed the test criterion with >80% correction rates in 20–40 sequential trials. This result demonstrated that Glra2 knockout mice had regular learning and motor abilities. Nevertheless, the visual acuity of Glra2 knockout mice was worse than that of their WT littermates (knockout: 0.55 cycles per degree (cpd) vs WT: 0.60 cpd, p<0.05, n=11 pairs) (figure 3A). We measured the mice RE according to the protocol by Schaeffel et al.32 Under dark adaptation, Glra2 knockout mice had regular pupil size (knockout: 2.52±0.04 mm, WT: 2.47±0.06 mm, p>0.05, n=8 pairs); however, they were more myopic than WT littermates (knockout: −3.92±1.34 D, WT: −0.50±0.72 D, p<0.05, n=8 pairs) (figure 3B).

Figure 3

Myopia-related phenotypes of Glra2 knockout (KO) mice. (A) Visual acuity of Glra2 knockout and wild-type (WT) mice. (B) Pupil size and refractive error of Glra2 KO and WT mice. (C) Normalised central corneal thickness of Glra2 KO and WT mice. (D) Dark-adapted electroretinography results of Glra2 KO and WT mice. (E) Statistical results of (D). Data are represented as mean±SEM. ns, not significant; *P<0.05; **P<0.01.

Glra2 knockout mice had reduced corneal thickness and dark-adapted electroretinography response

OCT experiments were performed to assess the ocular parameters of Glra2 knockout mice and to determine the origin of RE and visual acuity reduction. OCT results showed that Glra2 knockout mice had thinner corneas than their WT littermates (knockout: 0.1167±0.0037 mm, WT: 0.1259±0.0037 mm, p<0.05, n=8 pairs) (figure 3C). Conversely, other parameters such as corneal radius, chamber depth, lens thickness, vitreous depth, retinal thickness and axial length were not altered in Glra2 knockout mice (online supplemental figure 2A and online supplemental table 3). In addition, the thickness and stratification of the retina was similar in adult knockout and WT mice (online supplemental figure 2B,C).

We evaluated the retinal activity using ERG because GLRA2 is expressed in the retina and may play a role in the transmission of visual stimuli. After a dark adaption, Glra2 knockout mice presented decreased scotopic a and b waves and OPs wave amplitude (figure 3D–E). The photopic results revealed a reduced response to flash stimuli at both a and b and flicker wave amplitudes in knockout mice. However, the differences were not statistically significant (online supplemental figure 2D,E and online supplemental table 4). These results revealed a malfunction in rod pathway transduction exclusively in Glra2 knockout mice.

Glra2 defects hampered the retina rod cell genesis in vivo

We performed IHF assays on the retinas of P5.5 mice to assess rod genesis by staining the rod cell marker, rhodopsin. Glra2 defects dramatically decreased the rhodopsin-positive staining in the P5.5 mouse retina (figure 4A). To accurately evaluate the changes in cell differentiation, we calculated the proportion of rhodopsin-positive cells in primarily cultured retinal cells derived from P5.5 age mice after immunofluorescent staining with anti-rhodopsin. Rod cell genesis in Glra2 knockout mice decreased by approximately one-quarter (knockout: 19.32%, 95% CI 18.32% to 20.34%; p<0.001) compared with WT littermates (WT: 25.73%, 95% CI 24.68% to 26.79%) (figure 4B,C).

Figure 4

Immunohistofluorescence staining of mouse retina and immunofluorescent staining of primarily cultured retina cells. (A) Retina rod cell genesis in P5.5 age mice of each genotype. Immunohistofluorescence staining of paraffin sections from P5.5 age mouse retina; rod cells stained with anti-Rho are shown in red colour, and the nucleus is presented in blue. (B, C) Immunofluorescent staining and statistical results of the primarily cultured cells from P5.5 age mouse retina. Rho: Rhodopsin, a marker of the rod cell. The errors bar presents a 95% CI. ***P<0.001.

c.458G>A (p.Arg153Gln) and c.539G>T (p.Pro180Leu) variants disrupted GlyRα2 membrane location and agonist binding affinity

To evaluate the effects of the variants, we transfected HEK293 cells with WT, GLRA2R153Q, GLRA2P180L and GLRA2V341I plasmids. Immunofluorescent results showed that WT and GLRA2V341I proteins were expressed and located on the cell membranes with a scattered distribution. However, GLRA2R153Q and GLRA2P180L proteins were undetectable in the cell membrane (online supplemental figure 3A). Isolation of biotin-labelled membrane proteins also demonstrated that the membrane localisation of GLRA2R153Q and GLRA2P180L proteins was disrupted (online supplemental figure 3B).

As GlyRα2 is a membrane protein of the glycine-gated chloride channel family, we evaluated whether GLRA2R153Q and GLRA2P180L proteins could alter electrophysiological features through whole-cell patch experiments using HEK293 cells. As expected, the dose-response curves of GLRA2R153Q and GLRA2P180L shifted rightward compared with those of WT. Moreover, the EC50 value of glycine was significantly higher in GLRA2R153Q and GLRA2P180L than in WT (GLRA2R153Q: 11.550±0.666 mM, p<0.001; GLRA2P180L: 124.000±11.260 mM, p<0.001; WT: 0.083±0.010 mM). Meanwhile, GLRA2V341I only had a slightly elevated EC50 value (0.211±0.017 mM, p<0.001) compared with WT (online supplemental figure 3C). GLRA2R153Q and GLRA2P180L dramatically reduced GlyRα2 sensitivity to glycine and were unlikely to be activated in response to the physiological concentration of glycine.

Discussion

In this study, we identified the pathogenic variant c.539C>T (p.Pro180Leu) in GLRA2 gene, which co-segregated with HM in two unrelated Chinese families. The haplotype analysis showed no founder effects. These results indicated that c.539C>T was mutated separately in HM1 and HM2 families. We also found the pathogenic variant c.458G>A (p.Arg153Gln) in a patient with sporadic HM. In knockout mice, Glra2 deficiency caused myopia. This is the first evidence showing that GLRA2 gene can cause HM in humans and mice.

To date, no eye diseases caused by GLRA2 mutations have been reported.34 35 GLRA2 is highly expressed in the CNS and retina36 37; it encodes the α2 subunit of the glycine receptor GlyRα2, which is a ligand-gated chloride channel. In the adult mouse retina, GlyRα2 can enhance the excitatory centre response through crossover inhibition between the ON and OFF pathways,38 which is essential for the contrast encoding of visual stimuli.39 Besides myopia, we recorded the decrease of both dark-adapted ERG responses and corneal thickness in Glra2 knockout mice. Moreover, we observed hampered rod genesis in the Glra2 knockout mouse retina, in accordance with findings in vitro by Young and Cepko.40 GlyRα2 deficiency might cause insufficient photoperception and impaired visual transmission and processing, resulting in an altered visual experience. And the altered visual experience could ultimately lead to HM in both humans and mice.13 20 41

Variants c.458G>A (p.Arg153Gln) and c.539C>T (p.Pro180Leu) were absent in the gnomAD database and were highly conserved among many vertebrate animals (figure 1D). Arg153 is located in the first topological domain of GlyRα2 protein, while Pro180 is enveloped in the first cysteine loop domain of GlyRα2 protein (figure 1C). These domains are believed to play a crucial role in the agonist and antagonist binding and electrophysiological response.42 43 We found that both variants can disrupt the membrane location of GlyRα2. GLRA2R153Q and GLRA2P180L dramatically reduced GlyRα2 sensitivity to glycine, so that it would not be activated by the physiological concentration of glycine. These results indicated that c.458G>A and c.539C>T are pathogenic variants related to HM.

Notably, HM1-III:9 and HM2-II:2 subjects were both heterozygotes, which do not manifest HM. Therefore, the penetrance of the pathogenic variant c.539C>T in GLRA2 gene is incomplete (2/20), as observed in HM families. As GLRA2 is located on the X chromosome, we speculated that the incomplete penetrance of variant c.539C>T may be caused by skewed X-inactivation. However, we failed to detect any differences in the inactive proportion of X chromosomes between III:9 and other female patients in HM1 family using genomic DNA from peripheral blood lymphocyte (online supplemental figure 4). Thus, the causes of incomplete penetrance remain to be investigated in more dedicated studies. Moreover, a larger sample size is needed to depict the penetrance of c.539C>T in hemizygotes and the severity between hemizygotes and age-matched female heterozygotes.

Variant c.1021G>A (p.Val341Ile) is located in the topological domain between transmembrane domain 3 (TM3) and TM4 of GlyRα2 (figure 1C). This rare variant was found in the gnomAD database (1.09082e-05). This variant did not co-segregate with HM in HM3 family and did not affect GlyRα2’s membrane location, but had a slightly increased EC50 value. Considering that the glycine concentration at the synapses is estimated to be in the millimolar range,44 GLRA2V341I may normally respond to the physiological concentration. Therefore, c.1021G>A is not a pathogenic variant related to HM.

Variants in GLRA2 gene have been associated with autism disorders. Pinto reported an autistic patient with a 151 kb deletion in GLRA2 gene inherited from his mother. Notably, the patient, his mother, and his maternal grandfather had HM.35 45 Variant c.458G>A was also identified in an autistic boy (de novo mutation); however, the genotype of his autistic elder sister on this allele was WT.35 Additionally, three GLRA2 variants were reported in 2650 patients with autism; two were de novo and one was maternally inherited (online supplemental table 5).34 35 46 47 In the current study, sporadic and familial patients with GLRA2 variants exhibited normal social, behavioural and communication skills with personal contact. The phenotype caused by GLRA2 mutations was non-syndromic HM.

Our study had the following limitations: (1) the number of sporadic patients recruited was not large enough to evaluate the contribution of GLRA2 mutations to HM; (2) the causes of incomplete penetrance of c.539C>T (p.P180L) in female carriers and whether this phenomenon is common in male hemizygotes are unclear; (3) even though knockout mice showed myopia-related phenotypes, we failed to detect significant differences in axial elongation between Glra2 knockout and WT mice. According to Schmucker and Schaeffel,48 the −3.4 D RE change observed in our knockout mice would indicate a 19–23 µm axial elongation. The axial length of the WT mouse eye is approximately 3 mm, and it is difficult to obtain statistically significant results based on such a large baseline for such a small absolute alternation. Alternatively, the myopic RE in knockout mice may be attributed to corneal thinning other than elongated axial length49 50; (4) although it is evident that Glra2 knockout decreased rod cell genesis in the mouse retina, the mechanism underlying this phenomenon is unknown. Reduced cell proliferation, increased cell apoptosis and the downstream cascade caused by Glra2 knockout should be explored.

In summary, this study demonstrated that GLRA2 is a novel HM-causing gene and revealed the importance of extracellular glycine-gated chloride channels during HM onset and progression. In addition, this study added new evidence to previous suggestions that abnormal visual experience is a driver for HM and that ion channels are involved in this process.13 20 41 Nonetheless, more efforts should be made to elucidate the detailed HM pathogenic mechanism caused by GLRA2 mutations.

Data availability statement

All data relevant to the study are included in the article or uploaded as supplementary information. Not applicable.

Ethics statements

Patient consent for publication

Ethics approval

This study was approved by the Institutional Review Board of the School of Life Sciences, Central South University (2021-1-10). All subjects who participated in this study have thoroughly read and signed the informed consent form before blood samples were collected for further analysis.

Acknowledgments

We would like to thank Dr Jieqiong Tan for writing advice.

References

Supplementary materials

  • Supplementary Data

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Footnotes

  • Contributors Conceptualisation: QT, PT, KX, ZH; data curation: QT, RT, MD; formal analysis: QT, TC, GC, MD, RT; funding acquisition: ZH, QT, PT; investigation: QT, TC, GC, MD, RT, ZZ; methodology: QT, TC, GC, MD, RT, ZZ; resources: QT, PT, TC, ZH; supervision: QT, PT, KX, ZH; visualisation: QT, RT, MD; writing-original draft: QT, PT, KX, ZH; writing-review and editing: QT, PT, KX, ZH. ZH acting as guarantor.

  • Funding This study was supported by the Key R&D Program of Hunan Province (grant number 2019SK2051), National Key R&D Program of China (grant number 2021YFA0805200), the Natural Science Foundation of Hunan Province (grant number 2019JJ70002, 2021JJ40811 and 2021JJ30955), the Natural Science Foundation of Changsha City (grant number kq2014248).

  • Competing interests None declared.

  • Provenance and peer review Not commissioned; externally peer reviewed.

  • Supplemental material This content has been supplied by the author(s). It has not been vetted by BMJ Publishing Group Limited (BMJ) and may not have been peer-reviewed. Any opinions or recommendations discussed are solely those of the author(s) and are not endorsed by BMJ. BMJ disclaims all liability and responsibility arising from any reliance placed on the content. Where the content includes any translated material, BMJ does not warrant the accuracy and reliability of the translations (including but not limited to local regulations, clinical guidelines, terminology, drug names and drug dosages), and is not responsible for any error and/or omissions arising from translation and adaptation or otherwise.