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Article

A Dpagt1 Missense Variant Causes Degenerative Retinopathy without Myasthenic Syndrome in Mice

by
Lillian F. Hyde
1,†,
Yang Kong
1,2,†,
Lihong Zhao
1,
Sriganesh Ramachandra Rao
3,4,
Jieping Wang
1,
Lisa Stone
1,
Andrew Njaa
1,
Gayle B. Collin
1,
Mark P. Krebs
1,
Bo Chang
1,
Steven J. Fliesler
3,4,
Patsy M. Nishina
1 and
Jürgen K. Naggert
1,*
1
The Jackson Laboratory, Bar Harbor, ME 04609, USA
2
The Graduate School of Biomedical Science and Engineering, University of Maine, Orono, ME 04469, USA
3
Departments of Ophthalmology and Biochemistry and Neuroscience Graduate Program, Jacobs School of Medicine and Biomedical Sciences, State University of New York at Buffalo, Buffalo, NY 14203, USA
4
Research Service, VA Western New York Healthcare System, Buffalo, NY 14215, USA
*
Author to whom correspondence should be addressed.
†
These authors contributed equally to the work.
Int. J. Mol. Sci. 2022, 23(19), 12005; https://doi.org/10.3390/ijms231912005
Submission received: 29 July 2022 / Revised: 29 September 2022 / Accepted: 4 October 2022 / Published: 9 October 2022
(This article belongs to the Special Issue Novel Insights in Retinal Diseases Pathophysiology and Therapies)
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Abstract

:
Congenital disorders of glycosylation (CDG) are a heterogenous group of primarily autosomal recessive mendelian diseases caused by disruptions in the synthesis of lipid-linked oligosaccharides and their transfer to proteins. CDGs usually affect multiple organ systems and vary in presentation, even within families. There is currently no cure, and treatment is aimed at ameliorating symptoms and improving quality of life. Here, we describe a chemically induced mouse mutant, tvrm76, with early-onset photoreceptor degeneration. The recessive mutation was mapped to Chromosome 9 and associated with a missense mutation in the Dpagt1 gene encoding UDP-N-acetyl-D-glucosamine:dolichyl-phosphate N-acetyl-D-glucosaminephosphotransferase (EC 2.7.8.15). The mutation is predicted to cause a substitution of aspartic acid with glycine at residue 166 of DPAGT1. This represents the first viable animal model of a Dpagt1 mutation and a novel phenotype for a CDG. The increased expression of Ddit3, and elevated levels of HSPA5 (BiP) suggest the presence of early-onset endoplasmic reticulum (ER) stress. These changes were associated with the induction of photoreceptor apoptosis in tvrm76 retinas. Mutations in human DPAGT1 cause myasthenic syndrome-13 and severe forms of a congenital disorder of glycosylation Type Ij. In contrast, Dpagt1tvrm76 homozygous mice present with congenital photoreceptor degeneration without overt muscle or muscular junction involvement. Our results suggest the possibility of DPAGT1 mutations in human patients that present primarily with retinitis pigmentosa, with little or no muscle disease. Variants in DPAGT1 should be considered when evaluating cases of non-syndromic retinal degeneration.

1. Introduction

Congenital disorders of glycosylation (CDG) are a group of more than 160 rare genetic diseases [1,2,3,4], associated with more than 103 different genes [5], which are caused by defects in glycosylation [1,6]. Currently there are no cures and treatment is focused on reducing symptoms and improving quality of life [7]. In specific cases, dietary supplementation [8] or organ transplantation [9] may be helpful. A critical need in the path toward better treatments is the development of cell and animal models to better understand disease pathogenesis and to help develop drugs [5].
CDG Type 1 are a family of autosomal recessive diseases caused by defects in the synthesis of dolichol lipid-linked oligosaccharides and their transfer to proteins in the endoplasmic reticulum (ER) [10,11,12]. Currently there are 28 genes known to cause the disease (OMIM PS212065) whose presentation is highly variable, even within families that carry the same mutation [12,13,14]. In this study, we primarily focus on the role of a dolichol phosphate N-acetylglucosamine-1-phosphotransferase (DPAGT1) variant in the pathological events leading to retinal degeneration, which has yet to be fully elucidated.
The DPAGT1 gene encodes an integral ER membrane enzyme, which is ubiquitously expressed and catalyzes the first step of N-glycosylation [1], the predominant form of glycosylation in eukaryotes which governs protein folding and quality control [15]. Glycosylation is an essential process in growth and development, and the most common post-translational modification of lipids and proteins [16]. In human populations, DPAGT1 missense mutations are associated with limb girdle congenital myasthenic syndrome-13 (CMS13; OMIM 614750) and congenital disorders of glycosylation type Ij (CDG1J; OMIM 608093), both characterized by defects in cognitive and in motor abilities [17,18,19,20]. Retinal abnormalities, as a prominent pathological feature, are occasionally noted in CDG patients [21,22]. DPAGT1 is the primary mechanistic target of tunicamycin, a pharmacological agent which triggers secondary ER stress and the unfolded protein response (UPR) by blocking DPAGT1-dependent protein glycosylation [15,23]. Intravitreal injection of tunicamycin causes retinal degeneration driven by opsin hypoglycosylation [24,25], yet DPAGT1 function in the neural retina has not been thoroughly investigated.
Perhaps not surprisingly, given the critical role of DPAGT1 in glycosylation, null mutations in Dpagt1 lead to embryonic lethality in mice [26]. However, through the Translational Vision Research Models (TVRM) mutagenesis program [27,28], we identified a viable mouse line, tvrm76, which harbors a recessive D166G missense mutation in Dpagt1. The tvrm76 mutants were initially identified by a grainy fundus appearance with an attenuation of retinal vessels by indirect ophthalmoscopy. This clinical phenotype was associated with an early-onset photoreceptor degeneration, as assessed by histology. Biochemical characterization of the mutant revealed that increased ER stress may contribute to the cell death observed in the retina. The tvrm76 mutant is the first viable Dpagt1 model, and further study may provide additional insights into the role of glycosylation in retinal health and the mechanism through which Dpagt1tvrm76 mediates its effects on photoreceptor degeneration, serving as a unique model for investigating retinopathies reported in CDG patients.

2. Results

2.1. Homozygosity of the Dpagt1tvrm76 Allele Causes Early Onset Retinal Degeneration

Through screening of N-ethyl-N-nitrosourea (ENU) mutagenized C57BL/6J mice by indirect ophthalmoscopy, a strain with pronounced degenerative fundus changes, and progressive pigmentary retinopathy was observed and named tvrm76. In order to determine the molecular basis of the tvrm76 variant, linkage analysis was performed. A recessive locus associated with the retinopathy was identified on Chromosome 9 within an approximately 20 cM region between markers D9Mit129 and D9Mit11. Whole exome sequencing revealed a missense mutation in exon 3 of Dpagt1, in which adenine 497 is replaced by guanine (c.497A > G) (Figure 1A,B). The Dpagt1 mutation co-segregated with the degenerative fundus phenotype in backcross progeny, from the mapping cross, as determined by indirect ophthalmoscopy and by optical coherence tomography (OCT) (Figure 1E,F). The A > G nucleic acid transition is predicted to cause a substitution of an aspartic acid residue by glycine (D166G). By comparison with the 3D structure of human DPAGT1 (UniProt Q9H3H5), the mutated amino acid is located in an interfacial loop between transmembrane ⍺-helical segments 4 and 5 of the DPAGT1 protein, and is conserved among species (Figure 1C,D). Measuring Dpagt1 expression levels using qPCR showed a slight increase in expression in eyes of mice homozygous for the tvrm76 mutation relative to wild-type controls, however the difference between groups was not significant (Figure 1L).
In addition to the morphological characterization of the degenerative change, we also assessed retinal function in tvrm76 mice, using electroretinography (ERG) at one and three months of age. The scotopic a-wave and b-wave responses, associated primarily with rod photoreceptor function, were significantly impaired in one-month-old tvrm76 homozygotes in comparison to the wild-type littermates, and markedly deteriorated with age (Figure 1G,I,J). Likewise, photopic b-waves were also significantly compromised in tvrm76 homozygotes at three months of age (Figure 1H,K). The functional losses were concomitant with the observed loss of photoreceptors.

2.2. Rod Photoreceptor Specific Loss of DPAGT1 Function Causes Early Onset Retinal Degeneration

Understanding the role of Dpagt1 in vivo is difficult because null mutants are embryonic lethal [26]. To better characterize the effects of the Dpagt1tvrm76 mutation, we created two additional models (Figure 2A). The first, referred to as Rho iCre(+)-Dpagt1flox/flox, harbors a tissue specific knockout allele of Dpagt1 in rod photoreceptor cells, and was created by outcrossing a homozygous Dpagt1 floxed model, B6.129-Dpagt1tm2Jxm/J, with a transgenic mouse expressing rod photoreceptor-specific Cre recombinase, B6.Cg-Pde6b+ Tg(Rho-icre)1Ck/Boc (PMID15682388) and subsequently backcrossing Rho iCre(+)-Dpagt1flox/+ progeny to homozygous Dpagt1 floxed mice. The second model, referred to as Rho iCre(+)-Dpagt1flox/tvrm76, bears one conditional null allele of Dpagt1 and one Dpagt1tvrm76 allele.
To assess the phenotypic changes associated with the tvrm76 mutation, we performed fundoscopic examinations of tvrm76 homozygotes at one and three months of age, which showed a progressively grainy appearance, consistent with photoreceptor degeneration [29,30] (Figure 2B,C). Rho iCre(+)-Dpagt1flox/tvrm76 compound heterozygotes (Figure 2E,F) and Rho iCre(+)-Dpagt1flox/flox homozygotes (Figure 2H,I) displayed a more severe graininess, suggesting advanced degeneration by 3 months of age compared to Dpagt1tvrm76 homozygotes. This was consistent with our expectations that Dpagt1 is necessary for proper photoreceptor cell viability and function.

2.3. A Complementation Test Shows That the Dpagt1tvrm76 Mutation Causes the Retinal Degeneration

To confirm the causal relationship of the Dpagt1tvrm76 allele and the degenerative phenotype observed by funduscopy, we examined retinal histological sections from Dpagt1tvrm76 homozygotes, Rho iCre(+)-Dpagt1flox/tvrm76 compound heterozygotes, Rho iCre(+)-Dpagt1flox/flox homozygotes, and littermate wild-type controls at postnatal day 14, one month, and three months of age (Figure 3A). At three months of age, the compound heterozygotes had developed pronounced photoreceptor degeneration (Figure 3A), thus confirming that the mutation in Dpagt1tvrm76 leads to retinal degeneration in mice. Photoreceptor degeneration was assessed using the ratio of nuclei from the outer nuclear layer (ONL) to the inner nuclear layer (INL). Measurements were made at three distances from the optic nerve head central (500 µm, Supplementary Figure S1A), mid-peripheral (1000 µm, Figure 3B), and peripheral (1500 µm, Supplementary Figure S1A) to confirm that the effects were consistent across the retina. In the mid-peripheral sections (Figure 3), no differences in the ONL/INL ratio were observed among mutants and their wild-type controls at 14 days of age. At one month, only homozygous Dpagt1tvrm76 mutants showed significant degeneration in contrast to the compound heterozygotes Rho iCre(+)-Dpagt1flox/tvrm76 and homozygous Rho iCre(+)-Dpagt1flox/flox models, which were similar to wild-type littermates (Figure 3B). The peripheral retina appeared similar among all models at one month (Supplementary Figure S1A). Interestingly, by three months the compound heterozygotes and homozygous Rho iCre(+)-Dpagt1flox/flox mutants surpassed Dpagt1tvrm76 homozygotes in their degree of photoreceptor degeneration, with the homozygous Rho iCre(+)-Dpagt1flox/flox mutant having complete ONL loss (Figure 3B). The compound heterozygotes showed a significant thinning of photoreceptors, intermediate between the Dpagt1tvrm76 and Rho iCre(+)-Dpagt1flox/flox homozygotes in severity. The total loss of photoreceptors observed in the homozygous Rho iCre(+)-Dpagt1flox/flox model indicates that Dpagt1 is essential for ONL maintenance, and the slower rate of degeneration in tvrm76 indicates that the Dpagt1tvrm76 allele with the D166G mutation is hypomorphic and is likely to retain some function.

2.4. The Dpagt1tvrm76 Variant Is Not Associated with Aberrant Protein Glycosylation at an Early Age

DPAGT1 carries out the glycan tree transfer (oligosaccharyl transferase activity) in the N-linked glycosylation of proteins. Because many retinal proteins are normally glycosylated, their aberrant glycosylation might contribute to the degenerative retinopathy in Dpagttvrm76 homozygotes. However, qualitative examination of global glycosylation of retinal proteins by western blot analysis at two weeks and four weeks of age failed to show differences in glycosylation between homozygous Dpagttvrm76 and wild-type mice (Figure 4A,B).
Specific retinal proteins that undergo N-glycosylation include opsin. Opsin glycosylation defects lead to autosomal dominant retinitis pigmentosa [31,32,33]. Since it is conceivable that aberrant opsin glycosylation might contribute to the degenerative retinopathy in homozygous Dpagt1tvrm76 mice, we tested the N-glycosylation status of opsin. The glycosylation pattern of rhodopsin did not differ between mutants and wild-type at one month of age (Figure 4C). To increase the sensitivity of detecting hypomorphic effects of the Dpagttvrm76 allele on the N-linked glycosylation of rhodopsin, rhodopsin glycosylation was measured at two weeks of age in compound heterozygous (Rho iCre(+)-Dpagt1flox/tvrm76) mutants. Retinas from Tg(RHO*T17M)5Asl mice [34] served as a positive control, wherein opsin exhibited an electrophoretic mobility shift of ~1 kDa. Additionally, PNGase-F treated wild-type retinal protein lysate (to enzymatically deglycosylate proteins including opsin) served as a true positive control, wherein opsin exhibits a mobility shift of about 2 kDa, in agreement with previous findings [32]. Again, no difference was noted compared to the homozygous Dpagt1tvrm76 and wild-type controls (Figure 4C).

2.5. Homozgyous Dpagt1tvrm76 Mice Do Not Recapitulate Early Muscular Abnormalities Observed in Patients with DPAGT1 Mutations

Since DPAGT1 mutations are linked to congenital muscle weakness conditions in the human population, it prompted us to test whether Dpagt1tvrm76 homozygotes had muscle defects at a young age as well. A grip strength survey revealed a similar grip strength between Dpagt1tvrm76 homozygotes and their wild-type littermates at one month of age (Supplementary Figure S2A). Neuromuscular junctions in Dpagt1tvrm76 muscle tissue were also examined. Muscle whole mounts from Dpagt1tvrm76 mutants and controls were stained with anti-synaptophysin, which labels pre-synaptic vesicles, and with α-bungarotoxin (BTX) which binds the acetylcholine receptor (AchR) and localizes to the post-synapse of neuromuscular junctions. Our data showed a similar structural pattern of neuromuscular junctions in Dpagt1tvrm76 homozygotes and wild-type controls (Figure 4D). Transmission electron microscopy of the muscle did not show the tubular aggregates that are often seen in human patients with CMS [18] (Supplementary Figure S2B–E). Within the detection capacity of our assays, homozygous Dpagt1tvrm76 mice at a young age do not appear to recapitulate the early-onset myasthenic conditions associated with aberrant glycosylation in human patients.

2.6. Homozygous Dpagt1tvrm76 Eyes Show Signs of ER Stress

Since our results did not indicate significant defects in protein post-translational modification associated with the Dpagt1tvrm76 variant, we hypothesized that the activation of endoplasmic reticulum stress could mediate the mutation’s pathogenic effects. Defective glycosylation disrupts the normal post-translational modification of proteins and their proper maturation [35]. This disruption can affect the release of the abnormal proteins from the ER and lead to excessive protein accumulation and ER stress [36]. ER stress in turn can induce cell death [37,38,39]. To test if the mechanism underlying the photoreceptor degeneration in Dpagt1tvrm76 eyes might be attributable to a disturbance of ER homeostasis, a panel of ER-stress-associated molecules, including Hsp90b1 (Grp94), Hspa5 (Bip), Ddit3 (Chop), Atf4, and Padi2 (Pdi) were measured at the transcript level by qRT-PCR at two weeks of age, prior to the onset of photoreceptor degeneration (Figure 5A). Notably, Ddit3 was significantly upregulated in whole eyes of two-week-old animals. Hsp90b1 and Hspa5 also showed increased expression relative to wild-type littermate controls.
To localize ER stress within the retinal layers, immunofluorescent staining of HSPA5 (BiP) was carried out. Increased staining was observed in the inner nuclear layer (INL), retinal ganglion cell layer (RGC), and the photoreceptor inner segments of Dpagt1tvrm76 homozygotes were compared to the wild-type littermate controls (Figure 5B). The ER of photoreceptors is known to be localized in the inner segments, coinciding with our prediction of ER stress. Collectively, our observations revealed elevated transcript levels of some ER stress markers in tvrm76 mutant eyes that may be indicative of ER stress.

2.7. Increased Number of Apoptotic Cells Are Detected in Dpagt1tvrm76 Retinas

We next sought to determine the pathological consequences that might arise from ER stress. Considering the significant loss of photoreceptors in homozygous Dpagt1tvrm76 retinas, we examined whether cell-induced apoptosis was detectable by a TUNEL assay. A greater number of apoptotic cells were present in Dpagt1tvrm76 retinas compared to their wild-type counterparts at one month of age, which may underlie the observed loss of retinal cells (Figure 5C). The observation of TUNEL staining supports the initiation of cell apoptosis perhaps due to elevated ER stress, and substantiates retinal degeneration starting at a young age in Dpagt1tvrm76 homozygotes.

3. Discussion

The tvrm76 mutant was identified in an ENU mutagenesis screen, as a strain carrying a recessive mutation causing early-onset retinal degeneration. A missense mutation in Dpagt1 which is predicted to change aspartate 166 to glycine (D166G), was identified and its causative role in photoreceptor cell loss was confirmed by observing retinal degeneration in compound heterozygous, Rho+ Dpagt1flox/tvrm76, animals. The D166G mutation lies within the luminal loop between transmembrane segments 4 and 5 of the DPAGT1 protein, which contain residues predicted to interact with the dolichol-phosphate binding site. Furthermore, two severe CDGIj mutations in humans, L168P and Y170C, are localized in close proximity to D166G and retain only 25% of wild-type enzymatic activity [15]. Mutations occurring in these regions often significantly diminish catalytic activity of the molecule, whereas those that are distant from the active sites result in a smaller change in enzymatic activity [15,18,20,40,41]. In a qualitative assessment of glycosylation in homozygous Dpagt1tvrm76 eyes, we saw no noticeable difference in global and rhodopsin glycosylation at two and four weeks of age, respectively, similar to observations made in a model of rod photoreceptor-specific loss of DHDDS, an enzyme preceding DPAGT1 in the glycosylation chain [42]. In the case of Dpagt1tvrm76, it is, however, most likely that the D166G mutation represents a hypomorphic allele with sufficient activity to maintain near-normal glycosylation levels in the retina.
Dpagt1tvrm76 mutant mice may serve as a novel model for studying degenerative retinopathy due to defects associated with reduced DPAGT1 function. In clinics, many patients bearing mutations in DPAGT1 manifest multiple neurological symptoms [43,44,45,46]. Previous studies have primarily focused on the muscular presentations, while eye symptoms are rarely addressed [47,48,49,50]. In this study, we found that the Dpagt1tvrm76 model recapitulates the retinal degeneration found in some human patients and enables researchers to better probe the pathogenesis of degenerative changes in the retina caused by DPAGT1 mutations. Dpagt1 knockout mice are embryonic lethal [26,51], precluding the study of DPAGT1 in the retina. Therefore, the B6-Dpagt1tvrm76 and the rod photoreceptor-specific B6.129-Dpagt1tm2Jxm/J models provide a unique opportunity to study DPAGT1 function in this cell type. Future investigations using the rod photoreceptor-specific Dpagt1 deletion will facilitate the understanding of DPAGT1-dependent protein glycosylation in retinal development and/or maintenance.
Typically, patients harboring DPAGT1 variants present with limb-girdle weakness [52,53], and retinal degeneration is not noted. In this study, overt myasthenic manifestations were not detected in Dpagt1tvrm76 homozygotes. This is unlikely to be due to the specific affected isoform of DPAGT1, since all annotated splice variants carry the 166G mutant allele. While we only examined the grip strength of Dpagt1tvrm76 homozygotes at one-month of age, at six-months of age, the animals also did not show any apparent muscular weakness compared to the wild-type during normal ambulation. Additional examination at an advanced age would be desirable to assess potential long-term effects of the Dpagt1tvrm76 mutation on muscle function. It should be noted that a large number of patients harboring DPAGT1 variants were subject to underdiagnosis in clinics as well [45,52,53,54]. Nevertheless, our results demonstrate that Dpagt1 mutations exist which primarily present with an eye phenotype with minimal muscle involvement. It is possible that the observed phenotype depends on a combination of a specific allele and genetic background modifiers, especially since a variation in disease severity has been observed in human patients [50,52,55].
Proper glycosylation of a large array of proteins is important for their correct folding and stability [16,56,57,58]. Since glycosylation primarily occurs in the ER, accumulation of misfolded proteins there can result in ER stress and the induction of the unfolded protein response (UPR) [59,60,61]. The assessment of ER stress and UPR in human CDG has been carried out using patient-derived fibroblasts [20] and genetically engineered cell lines [62]. These experiments did not show an activation of UPR in fibroblasts carrying DPAGT1 mutations. However, the mutant cells were more sensitive to the ER stressor tunicamycin than control cells [20]. Concordantly, we observed only a moderate 30–70% increase in the expression levels of ER stress markers and a presence of HSPA5 (BiP)-positive cells in the eyes of homozygous Dpagt1tvrm76 mice. Whether this modest increase in ER stress, unfolded protein response, and DDIT3 (CHOP) activation is solely responsible for the observed apoptosis of photoreceptor cells in our model is currently unconfirmed.
The results presented here demonstrate that DPAGT1 mutations may exist which predominantly present at an early age as a non-syndromic retinal degeneration. DPAGT1 should, therefore, be considered as a candidate gene for retinal diseases which map within its vicinity. The Dpagt1tvrm76 model may be useful for pathological studies to better understand how a mutation in Dpagt1 leads to a retinal degenerative phenotype. In addition, the viability of Dpagt1tvrm76 makes it an attractive model for studying the role of DPAGT1 in other organ systems not examined in this study.

4. Materials and Methods

4.1. Mice, Mutagenesis, and Husbandry

All of the mice involved in this study were bred and housed in the Research Animal Facility at the Jackson Laboratory, and study protocols used in this project were reviewed and approved by the JAX Institutional Animal Care and Use Committee. Male C57BL/6J (B6/J, 000664) were mutagenized (G0) at 10–12 weeks of age by weekly intraperitoneal injections of N-ethylnitrosourea (Sigma-Aldrich, St. Louis, MO, USA) at 70 mg/kg body weight for three consecutive weeks. The G0 mice were mated with unmutagenized female B6/J to produce G1 progeny, which were subsequently mated to female B6/J to produce a G2 population. G2 females were backcrossed to their G1 sires to produce G3 mice, which were screened at 12 weeks for ocular phenotypes by indirect ophthalmoscopy. A G3 male mouse was found to have a fundus with grainy appearance. Because the G3 mouse did not breed, G3 siblings were intercrossed to confirm heritability and establish the line, named tvrm76 (C57BL/6J-Dpagt1tvrm76/Pjn), which showed recessive inheritance. From these initial matings, we determined that both homozygous tvrm76 male and female mice did not breed.
To conditionally knockout Dpagt1 in rod photoreceptors, mice bearing a Dpagt1-floxed allele, B6.129-Dpagt1tm2Jxm/J (JAX:006887), were crossed to B6.Cg-Pde6b+ Tg(Rho-icre)1Ck/Boc (JAX:015850) and backcrossed to generate mice homozygous for the floxed Dpagt1 allele and carrying the rod-expressing Rho-icre transgene (Rho iCre(+)-Dpagt1flox/flox).

4.2. Identification of the Molecular Basis of tvrm76

Due to the infertility of homozygous tvrm76 mutants, progeny-tested heterozygous mice were used in mapping experiments. C57BL/6J-Dpagt1tvrm76/Pjn heterozygotes were outcrossed to strain DBA/2J and resulting F1s were either backcrossed to C57BL/6J-Dpagt1tvrm76/Pjn heterozygotes or B6:D2-Dpagt1tvrm76 heterozygotes. In the former instance, only affected mice (grainy fundus) were used for linkage analysis. The chromosomal location of the tvrm76 locus was identified by genotyping 48 MIT markers across the genome in 24 affected mice from the linkage crosses. To identify the causative mutation, high-quality genomic DNA was prepared from the tails of tvrm76 homozygotes for the preparation of exome capture libraries which were sequenced on a HiSeq 2000 sequencing system (Illumina, San Diego, CA, USA), as previously described [63]. Whole-exome sequencing of tvrm76 identified a missense mutation in Dpagt1, which was subsequently confirmed by Sanger sequencing.

4.3. Phenotyping

The fundus of mouse eyes was examined using a Heine Omega 500 indirect ophthalmoscope with a 60-diopter aspheric lens [64]. Fundus images were captured using a Micron IV camera (Phoenix Research Laboratories, Vancouver, BC, Canada) after topical administration of 1% atropine sulphate for pupil dilation, and Goniovisc hypromellose ophthalmic solution (Sigma-Aldrich, St. Louis, MO, USA) for surface lubrication and the formation of a fluid bridge, as necessary [65]. Non-invasive sectional examination of mouse retinas was performed using a Bioptigen (Leica Microsystems, Deerfield, IL, USA) ultra-high resolution (UHR) Envisu R2210 spectral domain OCT (SDOCT) [65]. Mice eyes were dilated using 1% cyclopentolate (Akorn, Lake Forest, IL, USA) or 1% atropine (Akorn, Lake Forest, IL, USA) and anesthetized with ketamine/xylazine (100 mg/mL ketamine (Covetrus, Portland, ME, USA), 20 mg/mL xylazine (Akorn, Lake Forest, IL, USA), and 0.9% w/v sodium chloride). The function of the outer retina was assessed by electroretinography (ERG). Dpagt1tvrm76 homozygotes and their wild-type counterparts were examined at 1 and 3 months of age. ERG was recorded and analyzed following the routine protocol described previously [66]. Photoreceptor degeneration was assessed using the ratio of nuclei from the outer nuclear layer (ONL) to the inner nuclear layer (INL). Measurements were made at three distances from the optic nerve head central (500 µm), mid-peripheral (1000 µm), and peripheral (1500 µm) to confirm the effects were consistent across the retina. The measure of mouse grip strength was determined by recording the duration of time a mouse held onto an inverted wire mesh screen. The experiment followed a previously published protocol [67]. In brief, Dpagt1tvrm76 homozygotes and their wild-type control mice were placed in the center of a wire mesh screen, which was subsequently inverted (T0). The time when the mouse fell off was recorded (Tf).

4.4. Histology

For gross histology, eyes were enucleated from Dpagt1tvrm76 homozygotes and their sibling wild-type controls immediately after carbon dioxide asphyxiation. Tissues were fixed in acetic acid: methanol: phosphate buffer (1:3:4) prior to paraffin embedding and sectioning at 5 microns. Tissue sections were de-paraffinized and stained with hematoxylin and eosin (H and E staining), as previously described [66], and examined by light microscopy. Images were captured using a NanoZoomer 2.0-HT digital slide scanner (Hammamatsu, Shizuoka, Japan) at 40× magnification.

4.5. Electron Microscopy

Gastrocnemius muscle was fixed in a mixture of glutaraldehyde (2.5%) and paraformaldehyde (2%) in a sodium phosphate buffer. The samples were then post-fixed in 1% OsO4 and rinsed in a cacodylate buffer. After dehydration, tissue was embedded in Epon and sectioned for TEM cross-sectionally and longitudinally. Ultrastructure was imaged using a transmission electron microscope (Hitachi HT-7700, Tokyo, Japan).

4.6. RNA Extraction and Analysis

RNA was extracted from whole eyes of two-week-old Dpagt1tvrm76 and wild-type littermates using TRIzol (Invitrogen, Waltham, MA, USA, Cat #15596026) and the gentleMACS tissue dissociator (Miltenyi Biotec, Bergisch Gladbach, Germany, Cat #130-093-235). The mRNA was extracted using an RNeasy Mini Kit (Qiagen, Venlo, The Netherlands, Cat # 74104) following the protocol provided by the manufacturer. cDNA was synthesized using the SuperScript cDNA synthesis system (Invitrogen, Waltham, MA, USA, Cat #18091200), and q-RTPCR was performed using iTaq Universal SYBR Green Supermix in the CFX96 Touch Real-Time PCR Detection System (Bio-Rad, Hercules, CA, USA, Cat #1725121). The relative fold change was determined using the comparative CT method (ΔΔCt) and normalized to the level of ß-actin (Actb) mRNA, an internal control calibrator. The primers are presented in Supplementary Table S1.

4.7. Immunofluorescence

Enucleated eyes from two-week- and one-month-old Dpagt1tvrm76 mutants and wild-type littermates were fixed overnight in methanol:acetic acid in phosphate-buffered saline (PBS) at a ratio of 3:1:4. Tissues were subsequently embedded and sectioned at four µm for immunohistochemistry. Slides underwent a standard deparaffination and rehydration protocol. Antigen retrieval was performed using a 10 mM citrate buffer in a water bath set at 100 °C for 30 min. Nonspecific binding sites were blocked using 1:50 normal donkey serum (Jackson ImmunoResearch Laboratories, West Grove, PA, USA) and 0.5% Triton-X (Sigma-Aldrich, St. Louis, MO, USA) in PBS. Antibody incubation was performed, as previously described [66]. To prepare muscle specimens for whole-mount staining, tibialis anterior tissue was dissected and flattened immediately before overnight fixation with 4% paraformaldehyde (PFA, Sigma-Aldrich, St. Louis, MO, USA) in PBS at 4 °C. The muscle tissues were co-immunostained and mounted for imaging according to recommended procedures [68,69]. For detecting apoptotic cells, TUNEL assays were carried out by using the In Situ Apoptosis Detection, Alexa Fluor 647 Dye (Invitrogen, Cat #C10619), following the manufacturer’s protocol. Samples were mounted in Vectashield (Vector Laboratories, Burlingame, CA, USA) and imaged using a Zeiss Axio Observer.z1 fluorescence microscope (Carl Zeiss Microscopy, Jena, Germany). The resulting images were processed in Fiji (https://fiji.sc/#, accessed 3 October 2022) [70] using the Stack Focuser Macro.

4.8. Antibodies

Antibodies used for immunofluorescence staining included rabbit anti-GRP78 (1:200, Cell Signaling, Danvers, MA, USA, Cat #C50B12), fluorophore 594-conjugated α-Bungarotoxin (1:1000, Thermo Fisher Scientific, Waltham, MA, USA, Cat #B13423) and rabbit anti-synaptophysin (1:200, Abcam, Cambridge, UK, Cat #ab32127).

4.9. Western Blot

To assess global protein glycosylation, the Pro Q Emerald 488 Glycoprotein Stain Kit (Thermo Fisher Scientific, Waltham, MA, USA, Cat #P21875) was used to stain SDS-PAGE gels with Sypro Ruby, based on the manufacturer’s protocol. Immunoblot analysis for opsin glycosylation was carried out as described elsewhere [32]. Briefly, retinas from C57BL6/J, tvrm76 and Rho iCre(+)-Dpagt1flox/flox mice were harvested and flash frozen immediately. Retinas were lysed in RIPA buffer (Thermo Fisher Scientific, Waltham, MA, USA, Cat #89900) supplemented with protease inhibitor cocktail (ThermoFisher Scientific, Waltham, MA, USA, Cat #78441) at 1:100 dilution. Protein content in the lysates was estimated using a Pierce™ BCA Protein Assay Kit (ThermoFisher Scientific, Waltham, MA, USA, Cat #23225). Similarly processed RhoT17M/+ retinas served as a positive control for opsin hypo-glycosylation [34] (Tissues were a kind gift from Dr. Marina Gorbatyuk, UAB, Birmingham, AL, USA). PNGase-F N-glycosidase assay (New England Biolabs Inc., Ipswich, MA, USA; Cat #P0704S) was carried out as per the manufacturer’s instructions. About 20µg of C57BL6/J retinal protein lysate was treated with 200 U of PNGase-F in a 1X Glycobuffer 2 (10X buffer provided with the kit) supplemented with 1% NP-40 detergent at 37 °C, overnight. Protein lysates were subjected to Western blot analysis utilizing the following antibody mouse anti-opsin monoclonal antibody (Abcam, Burlingame, CA, USA; Cat #ab5417, 1:2000). Blots were then probed with appropriate host-specific alkaline phosphatase-tagged secondary antibodies (1 h at room temperature). Detection of antibody binding was achieved using chemifluorescent enzyme substrate (GE Healthcare Life Sciences, Marlborough, MA, USA; Cat #45000947) and a ChemiDoc™ MP Imaging System (Bio-Rad Laboratories, Hercules, CA, USA).

4.10. Image Analysis and Statistics

Fiji software (https://fiji.sc/#, accessed 3 October 2022) [70] was used for image processing and western blot quantification. Statistical significance was analyzed by two-way ANOVA with post hoc Bonferroni’s multiple comparisons test, or student-t test for comparisons of two groups using GraphPad Prism version 8 (GraphPad Software, San Diego, CA, USA). At least three biological replicates were utilized in each group for statistical analysis. Results are shown as mean ± SEM., p < 0.05 was reported as statistically significant.

Supplementary Materials

The following supporting information can be downloaded at: https://www.mdpi.com/article/10.3390/ijms231912005/s1.

Author Contributions

Conceptualization, P.M.N. and J.K.N.; methodology, L.Z., S.R.R., M.P.K. and S.J.F.; investigation, L.F.H., Y.K., G.B.C., L.Z., S.R.R., J.W., L.S., A.N. and M.P.K.; resources, L.S. and B.C.; writing—original draft preparation, L.F.H., Y.K. and L.Z.; writing—review and editing, L.F.H., Y.K., L.Z., S.R.R., A.N., G.B.C., M.P.K., B.C., S.J.F., P.M.N. and J.K.N.; visualization, L.F.H.; supervision, S.J.F., P.M.N. and J.K.N.; funding acquisition, S.R.R., B.C., S.J.F., P.M.N. and J.K.N. All authors have read and agreed to the published version of the manuscript.

Funding

Research in this publication was supported by the National Eye Institute of the National Institutes of Health under award numbers R01EY011996 to P.M.N., R01EY027305 to P.M.N. and M.P.K., R01EY019943 to B.C., and R01EY028561 to J.K.N., and by The Jackson Laboratory, Director’s Innovation Fund (DIF), award number 19000-13-12. SRR is the recipient of a Career Starter Research Grant Award from the Knights Templar Eye Foundation, Inc. SJF is the recipient of a Research Career Scientist Award (RCSA; IK6 BX005787) from the US Department of Veterans Affairs, BLR&D Service. Supported, in part, by facilities and resources provided by the VA Western NY Healthcare System (SJF, SRR). The authors also wish to acknowledge the support of the JAX Genome Technologies, Histopathology, and Microscopy Services, supported in part by the National Cancer Institute of the National Institutes of Health under award number P30CA034196.

Institutional Review Board Statement

The animal study protocol was approved by the JAX Institutional Animal Care and Use Committee (protocol ACUC 99089, last approved 22 August 2020).

Informed Consent Statement

Not applicable.

Data Availability Statement

Relevant data are contained within the article or Supplementary Materials. Additional datasets generated and/or analyzed for the current study are available from the corresponding author.

Acknowledgments

Illustrations were created with BioRender.com (https://biorender.com, accessed on 3 October 2022).

Conflicts of Interest

The authors declare no conflict of interest.

References

  1. Ng, B.G.; Freeze, H.H. Perspectives on Glycosylation and Its Congenital Disorders. Trends Genet. 2018, 34, 466–476. [Google Scholar] [CrossRef] [PubMed]
  2. Monticelli, M.; Francisco, R.; Brasil, S.; Marques-da-Silva, D.; Rijoff, T.; Pascoal, C.; Jaeken, J.; Videira, P.A.; Dos Reis Ferreira, V. Stakeholders’ views on drug development: The congenital disorders of glycosylation community perspective. Orphanet. J. Rare Dis. 2022, 17, 303. [Google Scholar] [CrossRef] [PubMed]
  3. Francisco, R.; Marques-da-Silva, D.; Brasil, S.; Pascoal, C.; Dos Reis Ferreira, V.; Morava, E.; Jaeken, J. The challenge of CDG diagnosis. Mol. Genet. Metab. 2019, 126, 1–5. [Google Scholar] [CrossRef] [PubMed]
  4. Freeze, H.H.; Jaeken, J.; Matthijs, G. CDG or not CDG. J. Inherit. Metab. Dis. 2022, 45, 383–385. [Google Scholar] [CrossRef] [PubMed]
  5. Peanne, R.; de Lonlay, P.; Foulquier, F.; Kornak, U.; Lefeber, D.J.; Morava, E.; Perez, B.; Seta, N.; Thiel, C.; Van Schaftingen, E.; et al. Congenital disorders of glycosylation (CDG): Quo vadis? Eur. J. Med. Genet. 2018, 61, 643–663. [Google Scholar] [CrossRef] [PubMed]
  6. Lefeber, D.J.; Freeze, H.H.; Steet, R.; Kinoshita, T. Congenital Disorders of Glycosylation. In Essentials of Glycobiology, 4th ed.; Varki, A., Cummings, R.D., Esko, J.D., Stanley, P., Hart, G.W., Aebi, M., Mohnen, D., Kinoshita, T., Packer, N.H., Prestegard, J.J., et al., Eds.; Cold Spring Harbor Laboratory Press: Cold Spring Harbor, NY, USA, 2022; pp. 599–614. Available online: https://www.ncbi.nlm.nih.gov/books/NBK579918/ (accessed on 3 October 2022).
  7. Park, J.H.; Marquardt, T. Treatment Options in Congenital Disorders of Glycosylation. Front. Genet. 2021, 12, 735348. [Google Scholar] [CrossRef] [PubMed]
  8. Boyer, S.W.; Johnsen, C.; Morava, E. Nutrition interventions in congenital disorders of glycosylation. Trends. Mol. Med. 2022, 28, 463–481. [Google Scholar] [CrossRef]
  9. Janssen, M.C.; de Kleine, R.H.; van den Berg, A.P.; Heijdra, Y.; van Scherpenzeel, M.; Lefeber, D.J.; Morava, E. Successful liver transplantation and long-term follow-up in a patient with MPI-CDG. Pediatrics 2014, 134, e279–e283. [Google Scholar] [CrossRef] [Green Version]
  10. Chang, I.J.; He, M.; Lam, C.T. Congenital disorders of glycosylation. Ann. Transl. Med. 2018, 6, 477–490. [Google Scholar] [CrossRef]
  11. Ondruskova, N.; Cechova, A.; Hansikova, H.; Honzik, T.; Jaeken, J. Congenital disorders of glycosylation: Still “hot” in 2020. Biochim. Biophys. Acta Gen. Subj. 2021, 1865, 129751. [Google Scholar] [CrossRef]
  12. Wilson, M.P.; Matthijs, G. The evolving genetic landscape of congenital disorders of glycosylation. Biochim. Biophys. Acta Gen. Subj. 2021, 1865, 129976. [Google Scholar] [CrossRef] [PubMed]
  13. Jaeken, J.; Lefeber, D.; Matthijs, G. Clinical utility gene card for: DPAGT1 defective congenital disorder of glycosylation. Eur. J. Hum. Genet. 2015, 23, 1749–1752. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  14. Selcen, D.; Shen, X.M.; Brengman, J.; Li, Y.; Stans, A.A.; Wieben, E.; Engel, A.G. DPAGT1 myasthenia and myopathy: Genetic, phenotypic, and expression studies. Neurology 2014, 82, 1822–1830. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  15. Dong, Y.Y.; Wang, H.; Pike, A.C.W.; Cochrane, S.A.; Hamedzadeh, S.; Wyszynski, F.J.; Bushell, S.R.; Royer, S.F.; Widdick, D.A.; Sajid, A.; et al. Structures of DPAGT1 Explain Glycosylation Disease Mechanisms and Advance TB Antibiotic Design. Cell 2018, 175, 1045–1058. [Google Scholar] [CrossRef]
  16. Schjoldager, K.T.; Narimatsu, Y.; Joshi, H.J.; Clausen, H. Global view of human protein glycosylation pathways and functions. Nat. Rev. Mol. Cell. Biol. 2020, 21, 729–749. [Google Scholar] [CrossRef] [PubMed]
  17. Paprocka, J.; Jezela-Stanek, A.; Tylki-Szymanska, A.; Grunewald, S. Congenital Disorders of Glycosylation from a Neurological Perspective. Brain Sci. 2021, 11, 88. [Google Scholar] [CrossRef]
  18. Belaya, K.; Finlayson, S.; Slater, C.R.; Cossins, J.; Liu, W.W.; Maxwell, S.; McGowan, S.J.; Maslau, S.; Twigg, S.R.; Walls, T.J.; et al. Mutations in DPAGT1 cause a limb-girdle congenital myasthenic syndrome with tubular aggregates. Am. J. Hum. Genet. 2012, 91, 193–201. [Google Scholar] [CrossRef] [Green Version]
  19. Belaya, K.; Finlayson, S.; Cossins, J.; Liu, W.W.; Maxwell, S.; Palace, J.; Beeson, D. Identification of DPAGT1 as a new gene in which mutations cause a congenital myasthenic syndrome. Ann. N. Y. Acad. Sci. 2012, 1275, 29–35. [Google Scholar] [CrossRef] [PubMed]
  20. Yuste-Checa, P.; Vega, A.I.; Martin-Higueras, C.; Medrano, C.; Gamez, A.; Desviat, L.R.; Ugarte, M.; Perez-Cerda, C.; Perez, B. DPAGT1-CDG: Functional analysis of disease-causing pathogenic mutations and role of endoplasmic reticulum stress. PLoS ONE 2017, 12, e0179456. [Google Scholar] [CrossRef] [Green Version]
  21. Messenger, W.B.; Yang, P.; Pennesi, M.E. Ophthalmic findings in an infant with phosphomannomutase deficiency. Doc. Ophthalmol. 2014, 128, 149–153. [Google Scholar] [CrossRef] [PubMed]
  22. Thompson, D.A.; Lyons, R.J.; Russell-Eggitt, I.; Liasis, A.; Jagle, H.; Grunewald, S. Retinal characteristics of the congenital disorder of glycosylation PMM2-CDG. J. Inherit. Metab. Dis. 2013, 36, 1039–1047. [Google Scholar] [CrossRef] [PubMed]
  23. Heifetz, A.; Keenan, R.W.; Elbein, A.D. Mechanism of action of tunicamycin on the UDP-GlcNAc: Dolichyl-phosphate GlcNAc-1-phosphate transferase. Biochemistry 1979, 18, 2186–2192. [Google Scholar] [CrossRef] [PubMed]
  24. Fliesler, S.J.; Basinger, S.F. Tunicamycin blocks the incorporation of opsin into retinal rod outer segment membranes. Proc. Natl. Acad. Sci. USA 1985, 82, 1116–1120. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  25. Fliesler, S.J.; Rapp, L.M.; Hollyfield, J.G. Photoreceptor-specific degeneration caused by tunicamycin. Nature 1984, 311, 575–577. [Google Scholar] [CrossRef] [PubMed]
  26. Marek, K.W.; Vijay, I.K.; Marth, J.D. A recessive deletion in the GlcNAc-1-phosphotransferase gene results in peri-implantation embryonic lethality. Glycobiology 1999, 9, 1263–1271. [Google Scholar] [CrossRef] [Green Version]
  27. Krebs, M.P.; Collin, G.B.; Hicks, W.L.; Yu, M.; Charette, J.R.; Shi, L.Y.; Wang, J.; Naggert, J.K.; Peachey, N.S.; Nishina, P.M. Mouse models of human ocular disease for translational research. PLoS ONE 2017, 12, e0183837. [Google Scholar] [CrossRef] [Green Version]
  28. Won, J.; Shi, L.Y.; Hicks, W.; Wang, J.; Hurd, R.; Naggert, J.K.; Chang, B.; Nishina, P.M. Mouse model resources for vision research. J. Ophthalmol. 2011, 2011, 391384. [Google Scholar] [CrossRef] [Green Version]
  29. Won, J.; Gifford, E.; Smith, R.S.; Yi, H.; Ferreira, P.A.; Hicks, W.L.; Li, T.; Naggert, J.K.; Nishina, P.M. RPGRIP1 is essential for normal rod photoreceptor outer segment elaboration and morphogenesis. Hum. Mol. Genet. 2009, 18, 4329–4339. [Google Scholar] [CrossRef] [Green Version]
  30. Chang, B.; Hawes, N.L.; Hurd, R.E.; Davisson, M.T.; Nusinowitz, S.; Heckenlively, J.R. Retinal degeneration mutants in the mouse. Vis. Res 2002, 42, 517–525. [Google Scholar] [CrossRef] [Green Version]
  31. Salom, D.; Jin, H.; Gerken, T.A.; Yu, C.; Huang, L.; Palczewski, K. Human red and green cone opsins are O-glycosylated at an N-terminal Ser/Thr–rich domain conserved in vertebrates. J. Biol. Chem. 2019, 294, 8123–8133. [Google Scholar] [CrossRef]
  32. Murray, A.R.; Vuong, L.; Brobst, D.; Fliesler, S.J.; Peachey, N.S.; Gorbatyuk, M.S.; Naash, M.I.; Al-Ubaidi, M.R. Glycosylation of rhodopsin is necessary for its stability and incorporation into photoreceptor outer segment discs. Hum. Mol. Genet. 2015, 24, 2709–2723. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  33. Berson, E.L.; Rosner, B.; Weigel-DiFranco, C.; Dryja, T.P.; Sandberg, M.A. Disease progression in patients with dominant retinitis pigmentosa and rhodopsin mutations. Investig. Ophthalmol. Vis. Sci. 2002, 43, 3027–3036. [Google Scholar]
  34. Nashine, S.; Bhootada, Y.; Lewin, A.S.; Gorbatyuk, M. Ablation of C/EBP homologous protein does not protect T17M RHO mice from retinal degeneration. PLoS ONE 2013, 8, e63205. [Google Scholar] [CrossRef] [PubMed]
  35. Michele, D.E.; Barresi, R.; Kanagawa, M.; Saito, F.; Cohn, R.D.; Satz, J.S.; Dollar, J.; Nishino, I.; Kelley, R.I.; Somer, H. Post-translational disruption of dystroglycan–ligand interactions in congenital muscular dystrophies. Nature 2002, 418, 417–421. [Google Scholar] [CrossRef] [PubMed]
  36. Rana, T.; Shinde, V.M.; Starr, C.R.; Kruglov, A.A.; Boitet, E.R.; Kotla, P.; Zolotukhin, S.; Gross, A.K.; Gorbatyuk, M.S. An activated unfolded protein response promotes retinal degeneration and triggers an inflammatory response in the mouse retina. Cell Death Dis. 2014, 5, e1578. [Google Scholar] [CrossRef] [Green Version]
  37. Tabas, I.; Ron, D. Integrating the mechanisms of apoptosis induced by endoplasmic reticulum stress. Nat. Cell Biol. 2011, 13, 184–190. [Google Scholar] [CrossRef] [Green Version]
  38. Wang, Q.; Wang, H.; Jia, Y.; Pan, H.; Ding, H. Luteolin induces apoptosis by ROS/ER stress and mitochondrial dysfunction in gliomablastoma. Cancer Chemother. Pharmacol. 2017, 79, 1031–1041. [Google Scholar] [CrossRef]
  39. Hu, H.; Tian, M.; Ding, C.; Yu, S. The C/EBP homologous protein (CHOP) transcription factor functions in endoplasmic reticulum stress-induced apoptosis and microbial infection. Front. Immunol. 2019, 9, 3083. [Google Scholar] [CrossRef] [Green Version]
  40. Li, H.; You, L.; Tian, Y.; Guo, J.; Fang, X.; Zhou, C.; Shi, L.; Su, Y.Q. DPAGT1-Mediated Protein N-Glycosylation Is Indispensable for Oocyte and Follicle Development in Mice. Adv. Sci. 2020, 7, 2000531. [Google Scholar] [CrossRef]
  41. Lehle, L.; Strahl, S.; Tanner, W. Protein glycosylation, conserved from yeast to man: A model organism helps elucidate congenital human diseases. Angew. Chem. Int. Ed. 2006, 45, 6802–6818. [Google Scholar] [CrossRef]
  42. Ramachandra Rao, S.; Skelton, L.A.; Wu, F.; Onysk, A.; Spolnik, G.; Danikiewicz, W.; Butler, M.C.; Stacks, D.A.; Surmacz, L.; Mu, X.; et al. Retinal Degeneration Caused by Rod-Specific Dhdds Ablation Occurs without Concomitant Inhibition of Protein N-Glycosylation. iScience 2020, 23, 101198. [Google Scholar] [CrossRef] [PubMed]
  43. Nicole, S.; Azuma, Y.; Bauche, S.; Eymard, B.; Lochmuller, H.; Slater, C. Congenital Myasthenic Syndromes or Inherited Disorders of Neuromuscular Transmission: Recent Discoveries and Open Questions. J. Neuromuscul. Dis. 2017, 4, 269–284. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  44. Engel, A.G.; Shen, X.M.; Selcen, D.; Sine, S.M. Congenital myasthenic syndromes: Pathogenesis, diagnosis, and treatment. Lancet Neurol. 2015, 14, 420–434. [Google Scholar] [CrossRef] [Green Version]
  45. Ng, B.G.; Underhill, H.R.; Palm, L.; Bengtson, P.; Rozet, J.M.; Gerber, S.; Munnich, A.; Zanlonghi, X.; Stevens, C.A.; Kircher, M.; et al. DPAGT1 Deficiency with Encephalopathy (DPAGT1-CDG): Clinical and Genetic Description of 11 New Patients. JIMD Rep. 2019, 44, 85–92. [Google Scholar]
  46. Engel, A.G. Genetic basis and phenotypic features of congenital myasthenic syndromes. Handb. Clin. Neurol. 2018, 148, 565–589. [Google Scholar]
  47. Issop, Y.; Hathazi, D.; Khan, M.M.; Rudolf, R.; Weis, J.; Spendiff, S.; Slater, C.R.; Roos, A.; Lochmüller, H. GFPT1 deficiency in muscle leads to myasthenia and myopathy in mice. Hum. Mol. Genet. 2018, 27, 3218–3232. [Google Scholar] [CrossRef] [Green Version]
  48. Gidaro, T.; Vandenbrande, L.; Malfatti, E.; Labasse, C.; Carlier, P.; Romero, N.; Servais, L.; Böhm, J. New homozygous mutation in DPAGT1 gene leading to LG-CMS with tubular aggregates. Neuromuscul. Disord. 2018, 28, S51. [Google Scholar] [CrossRef]
  49. Nicolau, S.; Kao, J.C.; Liewluck, T. Trouble at the junction: When myopathy and myasthenia overlap. Muscle Nerve 2019, 60, 648–657. [Google Scholar] [CrossRef]
  50. Bogdanova-Mihaylova, P.; Murphy, R.; Alexander, M.; McHugh, J.; Foley, A.R.; Brett, F.; Murphy, S. Congenital myasthenic syndrome due to DPAGT1 mutations mimicking congenital myopathy in an Irish family. Eur. J. Neurol. 2018, 25, e22–e23. [Google Scholar] [CrossRef]
  51. Kanaki, N.; Matsuda, A.; Dejima, K.; Murata, D.; Nomura, K.H.; Ohkura, T.; Gengyo-Ando, K.; Yoshina, S.; Mitani, S.; Nomura, K. UDP-N-acetylglucosamine-dolichyl-phosphate N-acetylglucosaminephosphotransferase is indispensable for oogenesis, oocyte-to-embryo transition, and larval development of the nematode Caenorhabditis elegans. Glycobiology 2019, 29, 163–178. [Google Scholar] [CrossRef]
  52. Finlayson, S.; Palace, J.; Belaya, K.; Walls, T.J.; Norwood, F.; Burke, G.; Holton, J.L.; Pascual-Pascual, S.I.; Cossins, J.; Beeson, D. Clinical features of congenital myasthenic syndrome due to mutations in DPAGT1. J. Neurol. Neurosurg. Psychiatry 2013, 84, 1119–1125. [Google Scholar] [CrossRef] [PubMed]
  53. Basiri, K.; Belaya, K.; Liu, W.W.; Maxwell, S.; Sedghi, M.; Beeson, D. Clinical features in a large Iranian family with a limb-girdle congenital myasthenic syndrome due to a mutation in DPAGT1. Neuromuscul. Disord. 2013, 23, 469–472. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  54. Estephan, E.P.; Zambon, A.A.; Thompson, R.; Polavarapu, K.; Jomaa, D.; Töpf, A.; Helito, P.V.; Heise, C.O.; Moreno, C.A.; Silva, A.M. Congenital myasthenic syndrome: Correlation between clinical features and molecular diagnosis. Eur. J. Neurol. 2022, 29, 833–842. [Google Scholar] [CrossRef] [PubMed]
  55. Citro, V.; Cimmaruta, C.; Monticelli, M.; Riccio, G.; Hay Mele, B.; Cubellis, M.V.; Andreotti, G. The analysis of variants in the general population reveals that PMM2 is extremely tolerant to missense mutations and that diagnosis of PMM2-CDG can benefit from the identification of modifiers. Int. J. Mol. Sci. 2018, 19, 2218. [Google Scholar] [CrossRef] [Green Version]
  56. Eichler, J. Protein glycosylation. Curr. Biol. 2019, 29, R229–R231. [Google Scholar] [CrossRef] [Green Version]
  57. Van Landuyt, L.; Lonigro, C.; Meuris, L.; Callewaert, N. Customized protein glycosylation to improve biopharmaceutical function and targeting. Curr. Opin. Biotechnol. 2019, 60, 17–28. [Google Scholar] [CrossRef]
  58. Esmail, S.; Manolson, M.F. Advances in understanding N-glycosylation structure, function, and regulation in health and disease. Eur. J. Cell Biol. 2021, 100, 151186. [Google Scholar] [CrossRef]
  59. Qi, Z.; Chen, L. Endoplasmic reticulum stress and autophagy. Autophagy Biol. Dis. 2019, 1206, 167–177. [Google Scholar]
  60. Choy, K.W.; Murugan, D.; Mustafa, M.R. Natural products targeting ER stress pathway for the treatment of cardiovascular diseases. Pharmacol. Res. 2018, 132, 119–129. [Google Scholar] [CrossRef]
  61. Medinas, D.B.; Rozas, P.; Traub, F.M.; Woehlbier, U.; Brown, R.H.; Bosco, D.A.; Hetz, C. Endoplasmic reticulum stress leads to accumulation of wild-type SOD1 aggregates associated with sporadic amyotrophic lateral sclerosis. Proc. Natl. Acad. Sci. USA 2018, 115, 8209–8214. [Google Scholar] [CrossRef] [Green Version]
  62. Lebedeva, I.V.; Wagner, M.V.; Sahdeo, S.; Lu, Y.-F.; Anyanwu-Ofili, A.; Matthew, B. Harms, M.B.; Wadia, J.S.; Rajagopal, G.; Boland, M.J.; et al. Precision genetic cellular models identify therapies protective against ER stress. Cell Death Dis. 2021, 12, 770–781. [Google Scholar] [CrossRef]
  63. Fairfield, H.; Gilbert, G.J.; Barter, M.; Corrigan, R.R.; Curtain, M.; Ding, Y.; D’Ascenzo, M.; Gerhardt, D.J.; He, C.; Huang, W.; et al. Mutation discovery in mice by whole exome sequencing. Genome Biol. 2011, 12, R86. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  64. Hawes, N.L.; Chang, B.; Hageman, G.S.; Nusinowitz, S.; Nishina, P.M.; Schneider, B.S.; Smith, R.S.; Roderick, T.H.; Davisson, M.T.; Heckenlively, J.R. Retinal degeneration 6 (rd6): A new mouse model for human retinitis punctata albescens. Invest. Ophthalmol. Vis. Sci. 2000, 41, 3149–3157. [Google Scholar] [PubMed]
  65. Krebs, M.P.; Xiao, M.; Sheppard, K.; Hicks, W.; Nishina, P.M. Bright-Field Imaging and Optical Coherence Tomography of the Mouse Posterior Eye. Methods Mol. Biol. 2016, 1438, 395–415. [Google Scholar] [PubMed]
  66. Kong, Y.; Zhao, L.; Charette, J.R.; Hicks, W.L.; Stone, L.; Nishina, P.M.; Naggert, J.K. An FRMD4B variant suppresses dysplastic photoreceptor lesions in models of enhanced S-cone syndrome and of Nrl deficiency. Hum. Mol. Genet. 2018, 27, 3340–3352. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  67. Takeshita, H.; Yamamoto, K.; Nozato, S.; Inagaki, T.; Tsuchimochi, H.; Shirai, M.; Yamamoto, R.; Imaizumi, Y.; Hongyo, K.; Yokoyama, S.; et al. Modified forelimb grip strength test detects aging-associated physiological decline in skeletal muscle function in male mice. Sci. Rep. 2017, 7, 42323. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  68. Burgess, R.W.; Cox, G.A.; Seburn, K.L. Neuromuscular disease models and analysis. Methods Mol. Biol. 2010, 602, 347–393. [Google Scholar] [PubMed]
  69. Motley, W.W.; Seburn, K.L.; Nawaz, M.H.; Miers, K.E.; Cheng, J.; Antonellis, A.; Green, E.D.; Talbot, K.; Yang, X.L.; Fischbeck, K.H.; et al. Charcot-Marie-Tooth-linked mutant GARS is toxic to peripheral neurons independent of wild-type GARS levels. PLoS Genet. 2011, 7, e1002399. [Google Scholar] [CrossRef] [PubMed]
  70. Schindelin, J.; Arganda-Carreras, I.; Frise, E.; Kaynig, V.; Longair, M.; Pietzsch, T.; Preibisch, S.; Rueden, C.; Saalfeld, S.; Schmid, B.; et al. Fiji: An open-source platform for biological-image analysis. Nat. Methods 2012, 9, 676–682. [Google Scholar] [CrossRef]
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Figure 1. Identification of the tvrm76 mutation and phenotypic characterization in the retina. (A) Genomic structure of Dpagt1. Whole exome sequencing revealed a missense mutation in exon 3 of Dpagt1 (E3, boxed in yellow) (B) The mutation results in a transition of adenine to guanine (c.497A > G, shaded in yellow) resulting in an amino acid substitution (aspartic acid (D) to glycine (G)) at residue 166. (C) DPAGT1 protein structure. Yellow arrow indicates location of variant domain. (D) Alignment of DPAGT1 amino acid sequences from different species around the tvrm76 variation. Blue arrow indicates location of D166G missense mutation. (E,F) A representative OCT image of a tvrm76 mutant compared to a wild-type (WT) littermate control. Double arrows indicate thickness of outer nuclear layer (ONL). INL, inner nuclear layer. (G–K) ERG recordings in tvrm76 mutants at 1 and 3 months of age. (G,I,J) Average scotopic rod response (flash stimuli: 0.25 cd.s/m2). (H,K) Average photopic cone response (flash stimuli: 10 cd.s/m2). Results are mean ± SEM. n = 5–9 **** p < 0.0001; ** p < 0.01; * p < 0.05 (Ordinary one-way ANOVA). (L) mRNA relative fold change (RFC) of Dpagt1 by qRT-PCR analysis. Results are mean ± SEM. n = 5 (p = 0.0819, Student t-test).
Figure 1. Identification of the tvrm76 mutation and phenotypic characterization in the retina. (A) Genomic structure of Dpagt1. Whole exome sequencing revealed a missense mutation in exon 3 of Dpagt1 (E3, boxed in yellow) (B) The mutation results in a transition of adenine to guanine (c.497A > G, shaded in yellow) resulting in an amino acid substitution (aspartic acid (D) to glycine (G)) at residue 166. (C) DPAGT1 protein structure. Yellow arrow indicates location of variant domain. (D) Alignment of DPAGT1 amino acid sequences from different species around the tvrm76 variation. Blue arrow indicates location of D166G missense mutation. (E,F) A representative OCT image of a tvrm76 mutant compared to a wild-type (WT) littermate control. Double arrows indicate thickness of outer nuclear layer (ONL). INL, inner nuclear layer. (G–K) ERG recordings in tvrm76 mutants at 1 and 3 months of age. (G,I,J) Average scotopic rod response (flash stimuli: 0.25 cd.s/m2). (H,K) Average photopic cone response (flash stimuli: 10 cd.s/m2). Results are mean ± SEM. n = 5–9 **** p < 0.0001; ** p < 0.01; * p < 0.05 (Ordinary one-way ANOVA). (L) mRNA relative fold change (RFC) of Dpagt1 by qRT-PCR analysis. Results are mean ± SEM. n = 5 (p = 0.0819, Student t-test).
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Figure 2. Generation and phenotypic characterization of tvrm76 and a rod photoreceptor-specific Dpagt1 conditional knockout by funduscopy. (A) Breeding schematic for tvrm76 and Dpagt1 conditional knockout models. tvrm76, a recessive RP model, was identified through a phenotype-driven screen of putative mutants (putants) generated by chemical mutagenesis (ENU) of C57BL/6J mice and subsequent intercrossing. For localized disruption of Dpagt1 in photoreceptors, Dpagt1tm2Jxm was bred with a transgenic mouse expressing rhodopsin-iCre. Subsequently Rho icre (+) Dpagt1flox/+ heterozygous progeny were backcrossed to homozygous Dpagt- floxed mice to generate Rho iCre(+)-Dpagt1flox/flox mice (Rho+ flox/flox). For allelic testing, Rho iCre(+)- Dpagt1flox/flox mice were crossed with a Dpagt1tvrm76 heterozygote to produce Rho iCre(+)-Dpagt1flox/tvrm76(Rho+ flox/tvrm76) compound heterozygotes. (B–J) Representative funduscopic images of central retina in mutant strains and controls at 1 and 3 months of age. (B,C) Dpagt1tvrm76 homozygotes, (D) wild-type (+/+) littermates. (E,F) Compound heterozygous (Rho+ flox/tvrm76), (H,I) Rho+ Dpagt1-floxed homozygotes and (G) Rho+ flox/+ and (J) Rho- flox/flox controls.
Figure 2. Generation and phenotypic characterization of tvrm76 and a rod photoreceptor-specific Dpagt1 conditional knockout by funduscopy. (A) Breeding schematic for tvrm76 and Dpagt1 conditional knockout models. tvrm76, a recessive RP model, was identified through a phenotype-driven screen of putative mutants (putants) generated by chemical mutagenesis (ENU) of C57BL/6J mice and subsequent intercrossing. For localized disruption of Dpagt1 in photoreceptors, Dpagt1tm2Jxm was bred with a transgenic mouse expressing rhodopsin-iCre. Subsequently Rho icre (+) Dpagt1flox/+ heterozygous progeny were backcrossed to homozygous Dpagt- floxed mice to generate Rho iCre(+)-Dpagt1flox/flox mice (Rho+ flox/flox). For allelic testing, Rho iCre(+)- Dpagt1flox/flox mice were crossed with a Dpagt1tvrm76 heterozygote to produce Rho iCre(+)-Dpagt1flox/tvrm76(Rho+ flox/tvrm76) compound heterozygotes. (B–J) Representative funduscopic images of central retina in mutant strains and controls at 1 and 3 months of age. (B,C) Dpagt1tvrm76 homozygotes, (D) wild-type (+/+) littermates. (E,F) Compound heterozygous (Rho+ flox/tvrm76), (H,I) Rho+ Dpagt1-floxed homozygotes and (G) Rho+ flox/+ and (J) Rho- flox/flox controls.
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Figure 3. Histological analysis of homozygous Dpagt1tvrm76 and homozygous Rho iCre(+)-Dpagt1flox/flox models shows progressive photoreceptor degeneration in the mid-periphery of the retina. (A) Hematoxylin and eosin (H and E stain) staining of posterior eye sections from Dpagt1tvrm76 homozygotes, compound heterozygotes (Rho+ flox/tvrm76) and homozygous Rho iCre(+)-Dpagt1flox/flox (Rho+ flox/flox) models at postnatal day 14 (p14), one month (1mo), and three months (3mo) and three month littermate controls. (B) Quantification of ONL nuclei degeneration relative to INL. Scale bar = 50 μm. Values represent mean ±SEM; n = 3–6. * p < 0.05; *** p < 0.001; **** p < 0.0001 (one-way ANOVA). IPL: inner plexiform layer; INL: inner nuclear layer; ONL: outer nuclear layer; RPE: retinal pigment epithelium.
Figure 3. Histological analysis of homozygous Dpagt1tvrm76 and homozygous Rho iCre(+)-Dpagt1flox/flox models shows progressive photoreceptor degeneration in the mid-periphery of the retina. (A) Hematoxylin and eosin (H and E stain) staining of posterior eye sections from Dpagt1tvrm76 homozygotes, compound heterozygotes (Rho+ flox/tvrm76) and homozygous Rho iCre(+)-Dpagt1flox/flox (Rho+ flox/flox) models at postnatal day 14 (p14), one month (1mo), and three months (3mo) and three month littermate controls. (B) Quantification of ONL nuclei degeneration relative to INL. Scale bar = 50 μm. Values represent mean ±SEM; n = 3–6. * p < 0.05; *** p < 0.001; **** p < 0.0001 (one-way ANOVA). IPL: inner plexiform layer; INL: inner nuclear layer; ONL: outer nuclear layer; RPE: retinal pigment epithelium.
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Figure 4. Protein glycosylation analysis in Dpagt1tvrm76 homozygotes. (A,B) No difference detected in total or glycosylated protein levels observed by SDS-PAGE analyses in Dpagt1tvrm76 homozygotes (2) and their wild-type (+/+) littermates (1) at four and two weeks of age. (C) Western blot of rhodopsin from Dpagt1tvrm76 homozygotes and compound heterozygotes (Rho+ flox/tvrm76) shows no glycosylation defect compared to the defect model and positive PNGase control at two weeks of age (n = 3). Asterisks indicate the 1 kDa shift for the opsin monomer (*) and the 2 kDa shift for the opsin dimer (**) after deglycosylation. (D) Immunostaining of muscle tissue whole mount (tibialis anterior) dissected from homozygous Dpagt1tvrm76 vs. +/+ against α-Synaptophysin (green) and α-Bungarotoxin (BTX, green). Scale bar = 5 μm.
Figure 4. Protein glycosylation analysis in Dpagt1tvrm76 homozygotes. (A,B) No difference detected in total or glycosylated protein levels observed by SDS-PAGE analyses in Dpagt1tvrm76 homozygotes (2) and their wild-type (+/+) littermates (1) at four and two weeks of age. (C) Western blot of rhodopsin from Dpagt1tvrm76 homozygotes and compound heterozygotes (Rho+ flox/tvrm76) shows no glycosylation defect compared to the defect model and positive PNGase control at two weeks of age (n = 3). Asterisks indicate the 1 kDa shift for the opsin monomer (*) and the 2 kDa shift for the opsin dimer (**) after deglycosylation. (D) Immunostaining of muscle tissue whole mount (tibialis anterior) dissected from homozygous Dpagt1tvrm76 vs. +/+ against α-Synaptophysin (green) and α-Bungarotoxin (BTX, green). Scale bar = 5 μm.
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Figure 5. Degenerative retinopathy as a possible consequence of ER-mediated stress response. (A) q-RTPCR analysis of ER stress-associated markers in homozygous Dpagt1tvrm76 vs. wild-type. Results mean ± SEM (n = 5). Student t-test; * p < 0.05; ** p < 0.01; *** p < 0.001. (B) Immunostaining of HSPA5 (BiP) (red) in Dpagt1tvrm76 homozygote vs. wild-type shows increased staining in the inner segments, INL, and RGC layers (white arrowheads). Blood vessel (white *). (C) TUNEL staining (purple) of cell apoptosis in the retina at fourteen days (p14) and one month (1mo) of age in Dpagt1tvrm76 homozygotes compared with wild-type. Arrows point to apoptotic cells. Boxed area in lower panel shows TUNEL staining (white) without DAPI. Scale bar (B,C) = 50 μm.
Figure 5. Degenerative retinopathy as a possible consequence of ER-mediated stress response. (A) q-RTPCR analysis of ER stress-associated markers in homozygous Dpagt1tvrm76 vs. wild-type. Results mean ± SEM (n = 5). Student t-test; * p < 0.05; ** p < 0.01; *** p < 0.001. (B) Immunostaining of HSPA5 (BiP) (red) in Dpagt1tvrm76 homozygote vs. wild-type shows increased staining in the inner segments, INL, and RGC layers (white arrowheads). Blood vessel (white *). (C) TUNEL staining (purple) of cell apoptosis in the retina at fourteen days (p14) and one month (1mo) of age in Dpagt1tvrm76 homozygotes compared with wild-type. Arrows point to apoptotic cells. Boxed area in lower panel shows TUNEL staining (white) without DAPI. Scale bar (B,C) = 50 μm.
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Hyde, L.F.; Kong, Y.; Zhao, L.; Rao, S.R.; Wang, J.; Stone, L.; Njaa, A.; Collin, G.B.; Krebs, M.P.; Chang, B.; et al. A Dpagt1 Missense Variant Causes Degenerative Retinopathy without Myasthenic Syndrome in Mice. Int. J. Mol. Sci. 2022, 23, 12005. https://doi.org/10.3390/ijms231912005

AMA Style

Hyde LF, Kong Y, Zhao L, Rao SR, Wang J, Stone L, Njaa A, Collin GB, Krebs MP, Chang B, et al. A Dpagt1 Missense Variant Causes Degenerative Retinopathy without Myasthenic Syndrome in Mice. International Journal of Molecular Sciences. 2022; 23(19):12005. https://doi.org/10.3390/ijms231912005

Chicago/Turabian Style

Hyde, Lillian F., Yang Kong, Lihong Zhao, Sriganesh Ramachandra Rao, Jieping Wang, Lisa Stone, Andrew Njaa, Gayle B. Collin, Mark P. Krebs, Bo Chang, and et al. 2022. "A Dpagt1 Missense Variant Causes Degenerative Retinopathy without Myasthenic Syndrome in Mice" International Journal of Molecular Sciences 23, no. 19: 12005. https://doi.org/10.3390/ijms231912005

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