Subjects

Abstract

Purpose

Using exome sequencing, the underlying variants in many persons with autosomal recessive diseases remain undetected. We explored autosomal recessive Stargardt disease (STGD1) as a model to identify the missing heritability.

Methods

Sequencing of ABCA4 was performed in 8 STGD1 cases with one variant and p.Asn1868Ile in trans, 25 cases with one variant, and 3 cases with no ABCA4 variant. The effect of intronic variants was analyzed using in vitro splice assays in HEK293T cells and patient-derived fibroblasts. Antisense oligonucleotides were used to correct splice defects.

Results

In 24 of the probands (67%), one known and five novel deep-intronic variants were found. The five novel variants resulted in messenger RNA pseudoexon inclusions, due to strengthening of cryptic splice sites or by disrupting a splicing silencer motif. Variant c.769-784C>T showed partial insertion of a pseudoexon and was found in cis with c.5603A>T (p.Asn1868Ile), so its causal role could not be fully established. Variant c.4253+43G>A resulted in partial skipping of exon 28. Remarkably, antisense oligonucleotides targeting the aberrant splice processes resulted in (partial) correction of all splicing defects.

Conclusion

Our data demonstrate the importance of assessing noncoding variants in genetic diseases, and show the great potential of splice modulation therapy for deep-intronic variants.

INTRODUCTION

In the past decade, next-generation sequencing (NGS) has enabled a rapid identification of novel disease genes,1,2,3 and transformed molecular diagnostic testing.4,5,6 Thus far, the emphasis was on coding and flanking splice site sequences that harbor the majority of genetic defects. Herewith, the underlying defects could be identified in ~50% of individuals with genetically heterogeneous diseases, including inherited retinal diseases (IRDs).7,8,9 Genome sequencing can identify the majority of noncoding sequence variants,1 but it will be very challenging to pinpoint the causal variants in the absence of assays that reveal the resulting messenger RNA (mRNA) and/or protein defects.

For diseases that are due to variants in a single gene, the yield of variants generally exceeds 50%. This is true for Stargardt disease (STGD1) (MIM 248200), which is caused by pathogenic variants in the gene encoding the adenosine triphosphate (ATP) binding cassette type A4 (ABCA4) (MIM 601691)10 as biallelic variants can be found in the majority of the cases11 and in a smaller proportion of other IRD subtypes.12,13,14 In ~30% of STGD1 cases, however, the expected second ABCA4 variant was lacking. A frequent coding variant, p.Asn1868Ile, was present in ~10% of STGD1 cases who had a severe pathogenic variant in trans and who generally showed late-onset disease.15,16 The remaining pathogenic variants in ABCA4 rarely consist of heterozygous deletions,17,18,19 whereas deep-intronic ABCA4 variants also account for some of the missing heritability in STGD1.11,17,20,21 By employing STGD1-derived keratinocytes, it was shown that some of these variants strengthen cryptic splice sites or create new splice sites, ultimately resulting in pseudoexon (PE) inclusions.21 Using STGD1-derived photoreceptor precursor cells (PPCs), we recently showed that two intronic variants in ABCA4 (c.4539+2001G>A and c.4539+2028C>T) strengthen exonic splice enhancer elements (ESEs), resulting in the inclusion of a 345-nt PE.22

PE inclusions due to deep-intronic variants are attractive targets for antisense oligonucleotide (AON)-based splicing correction.23 In the field of IRDs, these molecules have shown therapeutic potential for deep-intronic pathogenic variants in CEP290,24,25,26,27 USH2A,28 or OPA1,29 and a phase 1/2 clinical trial using AONs to treat CEP290-associated Leber congenital amaurosis is ongoing (NCT03140969).

In this study, we employed STGD1 as a model to assess the challenges to identify pathogenic noncoding variants. We sequenced the ABCA4 locus in 36 STGD1 individuals with one ABCA4 variant and p.Asn1868Ile in trans (n = 8), one ABCA4 variant (n = 25), or no (n = 3) ABCA4 variants. Selected noncoding variants were tested by in vitro splice assays or using STGD1-derived fibroblasts. Subsequently, several AONs were designed and successfully applied to redirect erroneous splicing.

MATERIALS AND METHODS

Samples

Written informed consent was obtained prior to participation in the study, which adhered to the Declaration of Helsinki. This study was approved by the Medical Ethical Committee 2010-359 (Protocol nr. 2009-32; NL nr. 34152.078.10) and the Commissie Mensgebonden Onderzoek Arnhem-Nijmegen (Dossier no. 2015-1543; dossier code sRP4h). More information regarding the proband cohort, and details of the materials and methods used, are provided in the Supplementary Material.


ABCA4 sequence analysis and selection of candidate splice variants

Detailed information of the selection of candidate splice variants and inclusion criteria is provided in the Supplementary Material.


Midigene-based splice assay

The effect of 11 noncoding variants was assessed by midigene-based splicing assays employing seven wild-type (WT) BA clones described previously30 and the newly designed BA30. WT and mutant constructs were transfected in HEK293T cells and the extracted total RNA was subjected to reverse transcription polymerase chain reaction (RT-PCR) (Table S1) as described previously.30


Single-molecule molecular inversion probe–based sequence analysis of intronic ABCA4 regions

To test the occurrence of five intronic ABCA4 variants (c.769-784C>T, c.859-506G>C, c.4253+43G>A, c.4539+1100A>G, c.4539+1106C>T) in 412 genetically unsolved STGD1 cases from France (n = 224) or Germany (n = 188), we designed single-molecule molecular inversion probes (smMIPs) based on a previously developed cost-effective sequencing protocol.31 The variant calling and annotation was performed using an in-house pipeline. The number of single-molecule consensus reads ranged from 14 to 1587, with an average coverage of 489x.


Antisense oligonucleotides

For each deep-intronic variant that caused PE inclusion, three AONs were designed (Table S2). The design of the therapeutic molecules was performed as described elsewhere.32 Oligonucleotides had a phosphorothioate backbone with a 2-O-methyl sugar modification (2OMe/PS) and were synthesized by Eurogentec. The oligonucleotides were resuspended in phosphate-buffered saline (PBS) and used at a concentration of 0.5 µM.


In vitro rescue studies in HEK293T cells using midigenes and AONs

HEK293T cells were transfected with either the wild-type or the mutant construct. Twenty-four hours posttransfection, each well was subdivided in five wells to be transfected with the respective AON, the sense oligonucleotide (SON), or left untransfected (NT). Forty-eight hours post-AON delivery, cells were harvested and RNA analysis was performed by RT-PCR. All experiments were performed in two independent replicates. Primer sequences can be found in Table S1.


Rescue studies using antisense oligonucleotides in fibroblasts

Fibroblast cells were transfected with each of the antisense oligonucleotides, or transfected with empty liposomes (NT). Forty-four hours posttransfection, medium was removed and medium containing cycloheximide (CHX) was added to block nonsense-mediated decay (NMD). Four hours later, cells were harvested and subjected to RNA analysis by RT-PCR. All experiments were performed in two independent replicates. Primer sequences are indicated in Table S1.


Capillary analysis

To quantify the ratios between correct and aberrant transcripts we loaded the RT-PCR samples onto a Fragment Analyzer Auto Capillary Electrophoresis System (Advanced Analytical Technologies, Inc.). Analysis of the peaks was performed using the corrected peak area parameter and only the peaks corresponding to the expected bands were taken into account.

RESULTS

Identification and selection of deep-intronic variants for splicing assay

Haloplex sequencing of eight STGD1 cases carrying one causal ABCA4 variant and p.Asn1868Ile in trans, 22 STGD1 cases with only one, and two cases carrying no ABCA4 variant, yielded 220 rare ABCA4 variants (allele frequency [AF] ≤0.01 in control individuals), consisting of 85 independent novel variants (Table S3). In the four British STGD1 cases with one (n = 3) or no (n = 1) ABCA4 variant analyzed by genome sequencing, eight novel rare (AF ≤0.01) independent ABCA4 variants remained (Table S3).

Eleven noncoding variants were selected for splice assays (Table S4). Seven of these (c.768+7329A>G, c.858+526T>G, c.859-506G>C, c.1555-5008C>T, c.4539+1100A>G, c.4539+1106C>T, c.6148-421T>C) were selected as they were located at cryptic splice sites or created a new putative splice site with a relative strength of at least 75% of the maximal score in two of five algorithms, and showed an increased splice prediction score of at least 2% (Table S4). Two variants, c.769-784C>T and c.4253+43G>A, belonging to three alleles (c.[769-784C>T; 5603A>T], c.[4253+43G>A; 6006-609T>A], c.[4253+43G>A; 5603A>T]), were enriched among the monoallelic cases, i.e., in 7 and 9 of 36 probands, respectively. The c.4253+43G>A variant was reported previously.33 Finally, the c.1937+435C>G variant was selected because it was located in the genomic sequence of an alternate exon in intron 13 (Chr1: 94,527,737–94,527,644).21

Four novel deep-intronic variants result in PE generation through the strengthening of splice sites

To test the functional effect of the 11 selected noncoding variants, seven ABCA4 wild-type midigene constructs previously described as BA4, BA6, BA7, BA9, BA11, BA19, and BA2130 and the newly designed BA30 (Table S5) were mutagenized. Upon RT-PCR and Sanger sequence validation, four variants had no effect (Figure S1). Variant c.858+526T>G did not show a PE insertion, but did yield four weak smaller fragments (Figure S1), the relevance of which is unknown in the absence of sequence results. This variant was found in cis with a complex allele containing a protein-truncating pathogenic variant (p.[Trp273*; Asn1868Ile]) in individual E-II:1, as determined by segregation analysis. The remaining six variants resulted in clear splice defects (Fig. 1, Figure S2) that allowed us to detect the second variant in 15/26 monoallelic probands, two deep-intronic variants in 2/3 cases without ABCA4 variants, and a complex allele (c.[769-784C>T; 5603A>T]) in seven STGD1 cases carrying one deep-intronic variant. Considering that these variants or complex alleles are causal, segregation was as expected (Table 1). The remaining 12 unsolved STGD1 cases are listed in Table S6.

Fig. 1
Fig. 1

Generation and assessment of splicing defects using midigenes. a Schematic representation of the five wild-type midigenes used that were cloned between exons 3 and 5 of Rhodopsin in pCI-Neo-RHO. Positions of the variants present in six mutant midigenes are indicated. b Assessment of the splicing defects upon midigene transfection in HEK293T cells. Five pseudoexon (PE) inclusions and one exon skipping event were detected in the mutant (MUT) constructs compared to the wild-type (WT). MQ stands for the negative control of the polymerase chain reaction (PCR). Rhodopsin (RHO) amplification was used as a transfection and loading control.

Table 1 Persons with Stargardt disease (STGD1) carrying two pathogenic ABCA4 alleles

The deep-intronic variant c.769-784C>T, present in 7/36 STGD1 cases, is located in intron 6, and was predicted to increase the strength of an intronic splice acceptor site at position g.94,549,775. In addition, a strong splice donor site was situated 161 nt downstream. RT-PCR analysis using wild-type and mutant minigene constructs revealed that, compared with the wild-type construct, the mutant c.769-784C>T construct showed an additional band of 296 bp, containing a 162-nt PE (Fig. 1b, Figure S2). Quantification of mutant mRNA in transfected HEK293T cells revealed that the PE fragment only accounted for ~8% of the total ABCA4 pre-mRNA (Table S7), suggesting a mild effect at the RNA and thus protein level (r.[=, 768_769ins(162)]; p.[=, Leu257Aspfs*3]).

The deep-intronic variant c.859-506G>C was predicted to significantly strengthen a cryptic intronic splice acceptor site and is accompanied by a downstream splice donor site. This variant resulted in a 56-nt PE insertion (Fig. 1b, Figure S2), which accounted for 75.5% of total splice products (Table S7), indicating the highly deleterious effect of this variant at the RNA and (predicted) protein level (r.[858_859ins(56), =]; p.[Phe287Thrfs*32, =]).

Deep-intronic variants c.4539+1100A>G and c.4539+1106C>T were predicted to alter the same cryptic splice donor site located at position g.94,493,901. A very strong splice acceptor site was located at g.94,493,968. Besides the expected 68-nt PE fragment (PE30.1) due to the splice acceptor site at position c.4539+1033 and the splice donor site at position c.4539+1100, an additional 112-nt PE (PE30.2) carrying the same splice donor but another acceptor site located at g.94,494,012 was observed (Fig. 1b, Figure S2). Interestingly, the relative ratios of these two PEs significantly differed between the midigene constructs carrying c.4539+1100A>G or c.4539+1106C>T. PE30.1 accounted for 60.6% and 93.1% of the total transcript in c.4539+1100A>G or c.4539+1106C>T respectively, while PE30.2 was present in 20.1% and 3.8% of the complementary DNA (cDNA) products, respectively (Table S7). Because both c.4539+1100A>G and c.4539+1106C>T showed only a minor fraction of correctly spliced products (19.2% and 3.0%) and because PE30.1 and PE30.2 are both predicted to lead to a frameshift, these variants were both deemed to have a severe effect (r.[4539_4540ins(68), 4539_4540ins(112), =]; p.[Arg1514Glyfs*3, Arg1514Valfs*31, =]) (Table 1, Table S8).

c.1937+435C>G results in PE generation through the disruption of putative splice silencers

The c.1937+435C>G variant did not alter the strength of a cryptic splice site. Instead, it was predicted to disrupt an ESE (SC35) motif, and, more importantly, to inactivate two splice silencer motifs and to lower the predicted strength of a third one (Figure S3). This variant was located within the genomic sequence of a low-abundance ABCA4 transcript that contains intron 13 sequences.21 RT-PCR analysis revealed a 134-nt PE insertion between positions c.1937+396 and c.1937+529 in mutant BA11 compared with WT (Fig. 1b, Figure S2). Although the splice defect caused by this variant disrupted the reading frame (r.[=, 1937_1938ins(134)]; p.[=, Ser646Serfs*25]), the fraction of mutant transcript was low (8.6%) (Table S7).

Variant c.4253+43G>A results in exon skipping through the disruption of putative splice silencers

The c.4253+43G>A variant was present in eight monoallelic STGD1 individuals and in one proband carrying a causal variant and p.Asn1868Ile in trans. It does not weaken the splice donor site of exon 28, nor does it affect any other cryptic splice sites in silico. It does affect the strength of several splice enhancer or silencer motifs (Figure S4). The c.4253+43G>A variant was found in cis with the previously reported c.6006-609T>A11 in eight of nine probands, but c.6006-609T>A showed no effect in an in vitro splice assay (Figure S2). The c.4253+43G>A mutant yielded bands of 495 and 370 bp, the first corresponding to the correctly spliced product, and the second to a product in which exon 28 was skipped (Fig. 1b, Figure S2). This 125-nt deletion is predicted to lead to a frameshift, and although both WT and mutant midigenes showed some skipping of exon 28, in the mutant construct this was significantly higher compared with WT (26.1% vs. 2.8%, Table S7). The fact that in all nine probands, a severe variant was found in trans, in combination with a late age of onset, suggests a mild effect of this variant (r.[=, 4129_4253del(125)]; p.[=, Ile1377Hisfs*3]). An overview of the allele frequencies and of the splice defects caused by all six variants can be found in Tables S8 and S9.

smMIP-based sequence analysis of intronic ABCA4 regions

Five of six intronic ABCA4 variants were analyzed for their recurrence in 412 genetically unsolved STGD1 cases from France (n = 224) or Germany (n = 188), by employing smMIPs.31 Three variants were found in a heterozygous state in this cohort: c.769-784C>T (n = 4), c.4253+43G>A (n = 29), and c.4539+1106C>T (n = 1) (Table S8 and Table S9), whereas variants c.859-506G>C and c.4539+1100A>G were not detected.

Antisense oligonucleotide-based exclusion of PEs

For five variants (c.769-784C>T, c.859-506G>C, c.1937+435C>G, c.4539+1100A>G, and c.4539+1106C>T), we designed three different AONs each that aim to result in PE exclusion. For c.4253+43G>A, only two AONs were designed, aiming to block splice silencer motifs to reinforce inclusion of exon 28. A summary of the sequences and characteristics of the AONs is provided in Table S2. The effect of the AONs at the RNA level was assessed by RT-PCR and subsequently semiquantified using capillary analysis (Figure S5, Table S7).

For c.769-784C>T, AON2 completely restored correct splicing, whereas AON3 had a partial effect (Fig. 2b). When using AON1, also some splice redirection was observed; an additional faint band was present both in WT and mutant. Cloning and sequence analysis of this band revealed that the 5’ 68 nt of the PE were skipped, while the 3’ 94 nt remained. Given the position of AON1, this AON most likely blocks the splice acceptor site of the PE, triggering the use of a downstream splice acceptor site. For c.859-506G>C, two AONs (AON1 and AON3) corrected the splicing defect (Fig. 2b). For c.1937+435C>G, all three AONs restored normal splicing (Fig. 2b). In addition, we observed that the 134-nt PE could also naturally be included in the WT construct, as the band was also present in the nontreated and the SON-treated samples. Since the PE is also inserted when transfecting the WT construct, the variant apparently enhances PE recognition. Finally, for the two neighboring variants c.4539+1100A>G and c.4539+1106C>T, AON1 and AON2 correctly restored splicing, while AON3 did not show any rescue (Fig. 2b).

Fig. 2
Fig. 2

Antisense oligonucleotide (AON) rescue using midigenes in HEK293T cells. a Position of the AONs and sizes of the pseudoexons introduced by the variants. b Assessment of the splicing correction by reverse transcription polymerase chain reaction (RT-PCR) upon AON delivery. Wild-type (WT) midigenes and mutant (MUT) midigenes were cotransfected with different AONs and a SON, except the nontransfected cells lane (NT). For each variant introducing a pseudoexon, at least one AON was able to redirect splicing. In the case of exon 28 skipping, a 10% inclusion was achieved with AON2. MQ denotes the negative control of the PCR reaction and HEK for the untransfected HEK293T. Rhodopsin (RHO) amplification was used as a transfection and loading control.

AON-based PE exclusion using STGD1-derived fibroblast cells

To investigate whether the AON-based splice corrections observed in the midigene assays would also occur in patient-derived cells, we generated fibroblast cell lines from a proband carrying c.[769-784C>T; 5603A>T] and c.1822T>A (p.Phe608Ile) (patient A-I:2), and from a STGD1 proband carrying c.859-506G>C and a putative deletion on the other allele encompassing intron 7 (case DNA14-33085; not listed in Table 1). For both cases, the same PEs were detected as in the midigene assays (Fig. 3), yet a larger amount of PE-containing mRNA was detected in fibroblasts from A-I:2 grown under NMD-suppressing conditions (18.2%) compared with HEK293T-transfected cells (8.6%). Considering that this STGD1 individual carries a missense variant (p.Phe608Ile), the amount of PE-containing mRNA from the c.769-784C>T allele likely is much higher than 18%. The same AONs that restored splicing in the midigenes also showed rescue in fibroblasts (Fig. 3). For c.769-784C>T, AON2 was the most effective, correcting 100% of the transcripts, whereas AON3 also showed a strong rescue (Fig. 3, Figure S6, Table S10). AON1 also resulted in PE skipping but induced an alternative splicing event. Interestingly, the insertion of this partial PE was also detected in control fibroblasts. Sequence analysis revealed that the upper band of the artifact corresponded to the partial PE, while the lower was a heteroduplex consisting of the WT and partial PE-containing transcripts. ABCA4 mRNA was also barely detected in the fibroblasts carrying c.859-506G>C when they were not subjected to CHX treatment (Fig. 3). After CHX incubation, a 56-nt PE was detected that, upon delivery of AON1 and AON3, was almost completely absent from the transcripts.

Fig. 3
Fig. 3

Antisense oligonucleotide (AON) rescue in fibroblasts derived from Stargardt disease (STGD1)-affected individuals carrying c.769-784C>T or c.859-506G>C. Fibroblast cells from a control (CON) and a STGD1 individual were transfected with three AONs and a SON. To detect the pseudoexon, cells were subjected to cycloheximide (+CHX) treatment. Only the nontransfected cells were not subjected to CHX treatment (-CHX). The MQ lane contains the negative control of the PCR reaction. Actin (ACTB) was used as a loading control.

AON-based exon inclusion

To correct the splice defect of c.4253+43G>A, AONs were designed to promote exon 28 inclusion. Two AONs were delivered to the midigene-transfected HEK293T cells. To assess whether the AON was inducing the inclusion of exon 28, the ratio between correct and Δexon 28 transcript was calculated with Fiji, or using the corrected peak area obtained in the capillary analysis (Figure S5). Using both methods, AON2 was shown to induce ~10% extra inclusion of exon 28 (Fig. 2), whereas for AON1, splice redirection was less evident (Table S7).

DISCUSSION

To identify missing noncoding variants in STGD1 cases, we sequenced the ABCA4 locus in 36 probands and identified one known and five novel intronic variants in 24 (67%) probands. Four novel deep-intronic variants (c.769-784C>T, c.859-506G>C, c.4539+1100A>G, c.4539+1106C>T) strengthen cryptic splice sites at noncanonical nucleotide positions and thereby result in PE insertions, contrary to most of the published deep-intronic splice site variants that create canonical splice sequences.34,35 Variant c.1937+435C>G disrupted a splicing silencer motif that is located within a low-expressed alternate exon, and resulted in a 134-nt PE formation.21 This PE contains a proper splice acceptor site but, similar to the alternate exon, no consensus splice donor site sequence. The c.4253+43G>A variant disrupted predicted splice silencers and created an ESE, and led to partial skipping of the upstream exon 28. Interestingly, we identified two probands (M-II:1 and P-II:3) that carried deep-intronic variants on both alleles.

All novel variants were predicted to result in protein truncation, but two variants, c.769-784C>T and c.4253+43G>A, found in seven and nine probands, respectively, only affect a small proportion of the mRNA. Testing of 412 other genetically unexplained STGD1 cases revealed 29 persons to carry c.4253+43G>A and four cases to carry c.769-784C>T. AONs were able to (partially) correct the observed splice defects for all variants in HEK293T cells and, for two variants, in STGD1-derived fibroblasts.

Fourteen first alleles in the 24 probands carry protein-truncating variants and are thus assumed to have a severe effect (Table 1). For other missense or complex alleles, the severity is less clear. Based on previous studies,15,36,37 our mRNA analysis of the deep-intronic variants, and the ages at onset of the STGD1 probands described here, we can hypothesize on the severity of the intronic variants. The c.859-506G>C, c.4539+1100A>G, and c.4539+1106C>T variants all show PE insertion in the majority of ABCA4 transcripts and can thus be considered severe variants. This correlates very well with an age at onset ≤10 years when found in trans with a severe variant and between 15 and 49 years when in trans with a mild variant (Table 1).

For c.1937+435C>G, the picture is more complicated. The splice defect was mild, and the two probands carrying this variant carry either a severe variant p.(Leu257Valfs*17) (U-II:1) or a mild allele p.[Gly863Ala, Gly863del; Asn1868Ile] (T-II:1) in trans. The ages of onset were 9 and 35 years, respectively, which argues for a severe nature of c.1937+435C>G in U-II:1 and a moderate-to-severe nature in T-II:1. This is discordant with the observed partial PE insertion in HEK293T cells. A similar observation was recently made while studying the effect of c.4539+2001G>A and c.4539+2028C>T.21 In STGD1-derived fibroblasts, mRNA analysis did not show any PE insertion. In STGD1-derived photoreceptor precursor cells however, we observed up to 15% (c.4539+2028C>T) and 25% (c.4539+2001G>A) of PE-containing mRNA.22 Based on their heterozygous presence in the corresponding STGD1 cases and their moderate-to-severe (c.4539+2028C>T) or severe (c.4539+2001G>A) nature, about two times these percentages were expected. We hypothesize that the photoreceptor precursor cells had not yet reached a differentiation stage that closely mimics the human retina situation. It is also of interest that, while c.1937+435C>G is predicted to disrupt ESEs, c.4539+2001G>A and c.4539+2028C>T are predicted to activate ESEs. Possibly, the action of these splicing motifs requires specific factors that are exclusively present in mature photoreceptors, while being absent in HEK293T cell and explain the small effect for c.1937+435C>G. Patient-derived photoreceptor-like cells may reveal a more complete splice defect.

Recently, it was determined that c.2588G>C (p.[Gly863Ala, Gly863del]) only acts as a penetrant pathogenic variant when present in cis with c.5603A>T (p.Asn1868Ile).15 The common p.(Asn1868Ile) variant was found as a second ABCA4 allele in up to 50% of monoallelic STGD1 cases and is strongly associated with late-onset STGD1.15 Upon Haloplex-based ABCA4 gene sequencing, we found p.Asn1868Ile as a single variant in trans with other (potentially) causal variants in 25/65 (38%) of probands, who had an average age at onset of 42 years. In addition, we identified four biallelic but unaffected persons and calculated that this variant, when present in trans with a loss-of-function ABCA4 variant, shows a penetrance <5%.16 Based on the relatively high frequency of c.769-784C>T in non-Finnish European controls (AF 0.00426 in gnomAD [http://gnomad.broadinstitute.org/]), its partial effect on splicing, and the very late age of onset observed in compound heterozygotes carrying c.[769-784C>T; 5603A>T] (61.0 years; range: 38–69 years), we consider that c.769-784C>T without c.5603A>T in cis may not be causative. We therefore investigated the MAFs of the c.769-784C>T and c.5603A>T variants (single and in combination) in 250 control Dutch families (GoNL: http://www.nlgenome.nl/).38 The single c.769-784C>T allele was found more often (6/998 alleles) than the c.[769-784C>T; 5603A>T] allele (2/998 alleles). The allele frequency of c.[769-784C>T; 5603A>T] in our STGD1 patient cohort (n = 250), 0.014, is significantly higher than in our general population (Chi-square test: p = 0.023; Bonferroni corrected). In two previous studies, the mean ages at onset for STGD1 patients carrying c.5603A>T as a single second allele in trans with severe ABCA4 variants were 36 years15 and 42 years.16 The mean age of onset for STGD1 patients carrying c.[769-784C>T; 5603A>T] is higher than the age of onset of patients carrying the single c.5603A>T variant (Mann–Whitney U; p<0.05). Given its relatively small effect on mRNA splicing (18.2% PE inclusion in mRNA from patient carrying this variant in a heterozygous manner) and its invariable cis-configuration with c.5603A>T, we cannot unequivocally assign pathogenicity to c.769-784C>T. Possibly, patient-derived photoreceptor progenitor cells may shed further light on this matter.

Interestingly, c.4253+43G>A also shows a relatively high non-Finnish European AF (0.00598 in gnomAD). Although c.4253+43G>A, with one exception (M-II:1), was found in cis with c.6006-609T>A, we did not observe a splice defect for the latter variant in vitro. This could be due to the lack of retina-specific splice factors in the tested cells or due to another missed deep-intronic variant that acts in concert with c.4253+43G>A. In the one proband with c.4253+43G>A who lacked c.6006-609T>A, the c.5603A>T (p.Asn1868Ile) variant was found in cis. The age of onset of the cases carrying c.4253+43G>A ranged from 18 to 61 years (average 41 years). Interestingly, the earliest age at onset (18 years) was observed in the proband M-II:1 who carried c.[4253+43G>A; 5603A>T].

The use of AONs to exclude PEs has been used for several IRD-associated genes.24,25,26,27,28,29 However, in this study, several technical challenges were observed. For the c.859-506G>C variant, the design of the AONs was limited to very small parts of the PE due to the repetitive nature of parts of the PE. In case of the c.4539+1100A>G and c.4539+1106C>T variants, we aimed to find effective AONs that would target the PE for both variants. In addition, using midigenes for c.769-784C>T, we observed variability between replicates, probably due to differences in the transfection efficiencies or passage of the cells. Nevertheless, for each variant, at least one effective AON was discovered.17

Despite the significant yield of novel ABCA4 variants in this study, a second ABCA4 variant was not detected in 11 monoallelic probands and there was one case with no ABCA4 variants, which could be due to (1) the presence of heterozygous copy-number variations (CNVs), as only three were tested using CNV analysis; (2) missed noncoding variants residing in noncovered sequences; (3) too-stringent selection criteria when using splicing algorithms; (4) incomplete sensitivity of the midigene in vitro splice assay; and (5) genocopies in view of the high AF of ABCA4 variants (5–10%) in the general population.18,36,39 Additional studies will be needed to further unravel the missing heritability of STGD1.

In conclusion, we identified deep-intronic variants in 24/36 (67%) of STGD1 cases with no ABCA4 variants, one variant, or one causal variant in trans with c.5603A>T. Two alleles (c.[769-784C>T; 5603A>T] and c.4253+43G>A) are frequent in our STGD1 cohort and appear to be associated with late-onset STGD1. Due to its small effect on ABCA4 mRNA in HEK293T cells and patient-derived fibroblasts, and its invariable presence on the same allele as c.5603A>T, we could not establish causality for c.769-784C>T. Interestingly, all the observed splice defects could be rescued with at least one of the tested AONs, which provides a basis for the development of new therapeutic strategies for individuals with STGD1 carrying these variants.

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Shared first authors: Riccardo Sangermano, Alejandro Garanto, Mubeen Khan

Shared senior: Rob W.J. Collin and Frans P.M. Cremers

References

  1. 1.

    Carss KJ, Arno G, Erwood M, et al. Comprehensive rare variant analysis via whole-genome sequencing to determine the molecular pathology of inherited retinal disease. Am J Hum Genet. 2017;100:75–90.

  2. 2.

    Ng SB, Turner EH, Robertson PD, et al. Targeted capture and massively parallel sequencing of 12 human exomes. Nature. 2009;461:272–276.

  3. 3.

    Nikopoulos K, Gilissen C, Hoischen A, et al. Next-generation sequencing of a 40 Mb linkage interval reveals TSPAN12 mutations in patients with familial exudative vitreoretinopathy. Am J Hum Genet. 2010;86:240–247.

  4. 4.

    Abu-Safieh L, Alrashed M, Anazi S, et al. Autozygome-guided exome sequencing in retinal dystrophy patients reveals pathogenetic mutations and novel candidate disease genes. Genome Res. 2013;23:236–247.

  5. 5.

    Beryozkin A, Shevah E, Kimchi A, et al. Whole exome sequencing reveals mutations in known retinal disease genes in 33 out of 68 Israeli families with inherited retinopathies. Sci Rep. 2015;5:13187.

  6. 6.

    Haer-Wigman L, van Zelst-Stams WA, Pfundt R, et al. Diagnostic exome sequencing in 266 Dutch patients with visual impairment. Eur J Hum Genet. 2017;25:591–599.

  7. 7.

    Gilissen C, Hehir-Kwa JY, Thung DT, et al. Genome sequencing identifies major causes of severe intellectual disability. Nature. 2014;511:344–347.

  8. 8.

    Neveling K, Feenstra I, Gilissen C, et al. A post-hoc comparison of the utility of Sanger sequencing and exome sequencing for the diagnosis of heterogeneous diseases. Hum Mutat. 2013;34:1721–1726.

  9. 9.

    Neveling K, Collin RW, Gilissen C, et al. Next-generation genetic testing for retinitis pigmentosa. Hum Mutat. 2012;33:963–972.

  10. 10.

    Allikmets R, Singh N, Sun H, et al. A photoreceptor cell-specific ATP-binding transporter gene (ABCR) is mutated in recessive Stargardt macular dystrophy. Nat Genet. 1997;15:236–246.

  11. 11.

    Zernant J, Xie YA, Ayuso C, et al. Analysis of the ABCA4 genomic locus in Stargardt disease. Hum Mol Genet. 2014;23:6797–6806.

  12. 12.

    Maugeri A, Klevering BJ, Rohrschneider K, et al. Mutations in the ABCA4 (ABCR) gene are the major cause of autosomal recessive cone-rod dystrophy. Am J Hum Genet. 2000;67:960–966.

  13. 13.

    Cremers FP, van de Pol DJ, van Driel M, et al. Autosomal recessive retinitis pigmentosa and cone-rod dystrophy caused by splice site mutations in the Stargardt's disease gene ABCR. Hum Mol Genet. 1998;7:355–362.

  14. 14.

    Fakin A, Robson AG, Fujinami K, et al. Phenotype and progression of retinal degeneration associated with nullizigosity of ABCA4. Invest Ophthalmol Vis Sci. 2016;57:4668–4678.

  15. 15.

    Zernant J, Lee W, Collison FT, et al. Frequent hypomorphic alleles account for a significant fraction of ABCA4 disease and distinguish it from age-related macular degeneration. J Med Genet. 2017;54:404–412.

  16. 16.

    Runhart EH, Sangermano R, Cornelis SS, et al. The common ABCA4 variant p.Asn1868Ile shows nonpenetrance and variable expression of Stargardt disease when present in trans with severe variants. Invest Ophthalmol Vis Sci. 2018;59:3220–3231.

  17. 17.

    Bax NM, Sangermano R, Roosing S, et al. Heterozygous deep-intronic variants and deletions in ABCA4 in persons with retinal dystrophies and one exonic ABCA4 variant. Hum Mutat. 2015;36:43–47.

  18. 18.

    Maugeri A, van Driel MA, van de Pol DJ, et al. The 2588G-->C mutation in the ABCR gene is a mild frequent founder mutation in the Western European population and allows the classification of ABCR mutations in patients with Stargardt disease. Am J Hum Genet. 1999;64:1024–1035.

  19. 19.

    Yatsenko AN, Shroyer NF, Lewis RA, Lupski JR. An ABCA4 genomic deletion in patients with Stargardt disease. Hum Mutat. 2003;21:636–644.

  20. 20.

    Bauwens M, De Zaeytijd J, Weisschuh N, et al. An augmented ABCA4 screen targeting noncoding regions reveals a deep intronic founder variant in Belgian Stargardt patients. Hum Mutat. 2015;36:39–42.

  21. 21.

    Braun TA, Mullins RF, Wagner AH, et al. Non-exomic and synonymous variants in ABCA4 are an important cause of Stargardt disease. Hum Mol Genet. 2013;22:5136–5145.

  22. 22.

    Albert S, Garanto A, Sangermano R, et al. Identification and rescue of splice defects caused by two neighboring deep-intronic ABCA4 mutations underlying Stargardt disease. Am J Hum Genet. 2018;102:517–527.

  23. 23.

    Hammond SM, Wood MJ. Genetic therapies for RNA mis-splicing diseases. Trends Genet. 2011;27:196–205.

  24. 24.

    Collin RW, den Hollander AI, van der Velde-Visser SD, Bennicelli J, Bennett J, Cremers FP. Antisense oligonucleotide (AON)-based therapy for Leber congenital amaurosis caused by a frequent mutation in CEP290. Mol Ther Nucleic Acids. 2012;1:e14.

  25. 25.

    Garanto A, Chung DC, Duijkers L, et al. In vitro and in vivo rescue of aberrant splicing in CEP290-associated LCA by antisense oligonucleotide delivery. Hum Mol Genet. 2016;25:2552–2563.

  26. 26.

    Gerard X, Perrault I, Hanein S, et al. AON-mediated exon skipping restores ciliation in fibroblasts harboring the common Leber congenital amaurosis CEP290 mutation. Mol Ther Nucleic Acids. 2012;1:e29.

  27. 27.

    Parfitt DA, Lane A, Ramsden CM, et al. Identification and correction of mechanisms underlying inherited blindness in human iPSC-derived optic cups. Cell Stem Cell. 2016;18:769–781.

  28. 28.

    Slijkerman RW, Vache C, Dona M, et al. Antisense oligonucleotide-based splice correction for USH2A-associated retinal degeneration caused by a frequent deep-intronic mutation. Mol Ther Nucleic Acids. 2016;5:e381.

  29. 29.

    Bonifert T, Gonzalez Menendez I, Battke F, et al. Antisense oligonucleotide mediated splice correction of a deep intronic mutation in OPA1. Mol Ther Nucleic Acids. 2016;5:e390.

  30. 30.

    Sangermano R, Khan M, Cornelis SS, et al. ABCA4 midigenes reveal the full splice spectrum of all reported noncanonical splice site variants in Stargardt disease. Genome Res. 2018;28:100–110.

  31. 31.

    Hiatt JB, Pritchard CC, Salipante SJ, O'Roak BJ, Shendure J. Single molecule molecular inversion probes for targeted, high-accuracy detection of low-frequency variation. Genome Res. 2013;23:843–854.

  32. 32.

    Garanto A, Collin RWJ. Design and in vitro use of antisense oligonucleotides to correct pre-mRNA splicing defects in inherited retinal dystrophies. Methods Mol Biol. 2018;1715:61–78.

  33. 33.

    Zernant J, Schubert C, Im KM, et al. Analysis of the ABCA4 gene by next-generation sequencing. Invest Ophthalmol Vis Sci. 2011;52:8479–8487.

  34. 34.

    Liquori A, Vache C, Baux D, et al. Whole USH2A gene sequencing identifies several new deep intronic mutations. Hum Mutat. 2016;37:184–193.

  35. 35.

    Vaz-Drago R, Custodio N, Carmo-Fonseca M. Deep intronic mutations and human disease. Hum Genet. 2017;136:1093–1111.

  36. 36.

    Cornelis SS, Bax NM, Zernant J, et al. In silico functional meta-analysis of 5,962 ABCA4 variants in 3,928 retinal dystrophy cases. Hum Mutat. 2017;38:400–408.

  37. 37.

    Zhang N, Tsybovsky Y, Kolesnikov AV, et al. Protein misfolding and the pathogenesis of ABCA4-associated retinal degenerations. Hum Mol Genet. 2015;24:3220–3237.

  38. 38.

    Genome of the Netherlands Consortium. Whole-genome sequence variation, population structure and demographic history of the Dutch population. Nat Genet. 2014;46:818–825.

  39. 39.

    Jaakson K, Zernant J, Kulm M, et al. Genotyping microarray (gene chip) for the ABCR (ABCA4) gene. Hum Mutat. 2003;22:395–403.

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Acknowledgements

We thank Ellen Blokland, Lonneke Duijkers, Duaa Elmelik, Anita Hoogendoorn, Marlie Jacobs-Camps, Saskia van der Velde-Visser, and Marijke Zonneveld-Vrieling for technical assistance. We thank Sabine Defoort, Hélène Dollfus, Isabelle Drumare, Christian P. Hamel, Karsten Hufendiek, Cord Huchzermeyer, Herbert Jägle, Ulrich Kellner, Philipp Rating, Klaus Rüther, Eric Souied, Georg Spital, and Xavier Zanlonghi for their cooperation and ascertaining STGD1 cases. This work was supported by the FP7-PEOPLE-2012-ITN programme EyeTN, agreement 317472 (to F.P.M.C.); the Macula Vision Research Foundation (to F.P.M.C.); the Foundation Fighting Blindness USA, grant no. PPA-0517-0717-RAD (to A.G., C.B.H., F.P.M.C., R.W.J.C., and S.A.); the RP Fighting Blindness UK (RetinaUK), grant no. GR591 (to F.P.M.C. and S.A.); the Rotterdamse Stichting Blindenbelangen, the Stichting Blindenhulp, and the Stichting tot Verbetering van het Lot der Blinden (to F.P.M.C. and S.A.); and by the Landelijke Stichting voor Blinden en Slechtzienden, Macula Degeneratie fonds, and the Stichting Blinden-Penning, which contributed through Uitzicht 2016-12 (to F.P.M.C. and S.A.). This work was also supported by the Algemene Nederlandse Vereniging ter Voorkoming van Blindheid, Stichting Blinden-Penning, Landelijke Stichting voor Blinden en Slechtzienden, Stichting Oogfonds Nederland, Stichting Macula Degeneratie Fonds, and Stichting Retina Nederland Fonds, which contributed through UitZicht 2015-31, together with the Rotterdamse Stichting Blindenbelangen, Stichting Blindenhulp, Stichting tot Verbetering van het Lot der Blinden, Stichting voor Ooglijders, and Stichting Dowilvo (to A.G. and R.W.J.C.); the Stichting Macula Degeneratie Fonds; and the Stichting A.F. Deutman Researchfonds Oogheelkunde (to C.B.H.). This work was also supported by the Algemene Nederlandse Vereniging ter Voorkoming van Blindheid and Landelijke Stichting voor Blinden en Slechtzienden, which contributed through UitZicht 2014-13, together with the Rotterdamse Stichting Blindenbelangen, Stichting Blindenhulp, and the Stichting tot Verbetering van het Lot der Blinden (to F.P.M.C.), the Ghent University Research Fund (BOF15/GOA/011), the Research Foundation Flanders (FVO) G0C6715N, and the Hercules Foundation AUGE/13/023 and JED Foundation to E.D.B. M.B. was PhD fellow of the FWO and recipient of a grant of the funds for Research in Ophthalmology (FRO). E.D.B. is Senior Clinical Investigator of the FWO (1802215N). This work was also supported by the National Institute for Health Research (NIHR) Biomedical Centre at Moorfields and UCL Institute of Ophthalmology (to A.W.), UK NIHR Rare Disease Translational Research Consortium (to G.A. and A.W.), NIHR for the NIHR BioResource (RG65966) (to F.L.R.) by grants from the Federal Ministry of Education and Research (BMBF) (ref. IDs 01GM0851 and 01GM1108B) (to B.H.F.W.). G.A. is supported by a Fight for Sight UK Early Career Investigator Award. The funding organizations had no role in the design or conduct of this research, and provided unrestricted grants. This study made use of data generated by the Genome of the Netherlands Project. Funding for the project was provided by the Netherlands Organization for Scientific Research under award number 184021007, dated 9 July 2009 and made available as a Rainbow Project of the Biobanking and Biomolecular Research Infrastructure Netherlands (BBMRI-NL). Samples where contributed by LifeLines (http://lifelines.nl/lifelines-research/general), the Leiden Longevity Study (http://www.healthy-ageing.nl; http://www.langleven.net), the Netherlands Twin Registry (NTR: http://www.tweelingenregister.org), the Rotterdam studies (http://www.erasmus-epidemiology.nl/rotterdamstudy), and the Genetic Research in Isolated Populations program (http://www.epib.nl/research/geneticepi/research.html#gip). The sequencing was carried out in collaboration with the Beijing Institute for Genomics (BGI).

Author information

Affiliations

  1. Department of Human Genetics, Radboud University Medical Center, Nijmegen, The Netherlands

    • Riccardo Sangermano PhD
    • , Alejandro Garanto PhD
    • , Mubeen Khan MSc
    • , Muhammad Imran Khan PhD
    • , Stéphanie S. Cornelis MSc
    • , Silvia Albert PhD
    • , Rob W. J. Collin PhD
    •  & Frans P. M. Cremers PhD
  2. Radboud Institute for Molecular Life Sciences, Radboud University Medical Center, Nijmegen, The Netherlands

    • Riccardo Sangermano PhD
    •  & Muhammad Imran Khan PhD
  3. Donders Institute for Brain, Cognition and Behaviour, Radboud University Medical Center, Nijmegen, The Netherlands

    • Alejandro Garanto PhD
    • , Mubeen Khan MSc
    • , Esmee H. Runhart MD
    • , Nathalie M. Bax MD
    • , Stéphanie S. Cornelis MSc
    • , Carel B. Hoyng MD, PhD
    • , Silvia Albert PhD
    • , Rob W. J. Collin PhD
    •  & Frans P. M. Cremers PhD
  4. Department of Ophthalmology, Radboud University Medical Center, Nijmegen, The Netherlands

    • Esmee H. Runhart MD
    • , Nathalie M. Bax MD
    • , Caroline C. W. Klaver MD, PhD
    •  & Carel B. Hoyng MD, PhD
  5. Center for Medical Genetics, Ghent University and Ghent University Hospital, Ghent, Belgium

    • Miriam Bauwens PhD
    • , Sarah Naessens MSc
    •  & Elfride De Baere MD, PhD
  6. The Rotterdam Eye Hospital and the Rotterdam Ophthalmic Institute, Rotterdam, The Netherlands

    • L. Ingeborgh van den Born MD, PhD
  7. Department of Medical Genetics, University Medical Center Groningen, University of Groningen, Groningen, The Netherlands

    • Joke B. G. M. Verheij MD
  8. Department of Ophthalmology, University Medical Center Groningen, University of Groningen, Groningen, The Netherlands

    • Jan-Willem R. Pott MD, PhD
  9. Department of Ophthalmology, Erasmus Medical Center, Rotterdam, The Netherlands

    • Alberta A. H. J. Thiadens MD, PhD
    •  & Caroline C. W. Klaver MD, PhD
  10. Service d′Exploration de la Vision CHU, Lille, France

    • Bernard Puech MD
  11. Institute for Neurosciences of Montpellier INSERM U1051, University of Montpellier, Montpellier, France

    • Isabelle Meunier PhD
  12. Centre d′Etude du Polymorphisme Humain, Fondation Jean Dausset, Paris, France

    • Isabelle Meunier PhD
  13. UCL Institute of Ophthalmology, London, UK

    • Gavin Arno PhD
    • , Ana Fakin PhD
    •  & Andrew R. Webster MD, PhD
  14. Moorfields Eye Hospital, London, UK

    • Gavin Arno PhD
    • , Ana Fakin PhD
    •  & Andrew R. Webster MD, PhD
  15. Department of Haematology, University of Cambridge, Cambridge, UK

    • Keren J. Carss PhD
  16. NIHR BioResource, Cambridge University Hospitals NHS Foundation Trust, Cambridge Biomedical Campus, Cambridge, UK

    • Keren J. Carss PhD
    •  & F. Lucy Raymond MD, PhD
  17. Department of Medical Genetics, Cambridge Institute for Medical Research, University of Cambridge, Cambridge, UK

    • F. Lucy Raymond MD, PhD
  18. Univ. Lille, Inserm UMR-S 1172, CHU Lille, Biochemistry and Molecular Biology Department - UF Génopathies, Lille, France

    • Claire-Marie Dhaenens MD, PhD
  19. Institut für Humangenetik, Universität Regensburg, Regensburg, Germany

    • Heidi Stöhr PhD
    • , Felix Grassmann PhD
    •  & Bernhard H. F. Weber PhD
  20. Department of Medical Epidemiology and Biostatistics, Karolinska Institutet, Stockholm, Sweden

    • Felix Grassmann PhD

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Disclosure

R.W.J.C., A.G., F.P.M.C., and S.A. are inventors on one or two filed patents (nos. 16203864.0 and 18184432.5) that are related to the contents of this manuscript. The other authors declare no conflicts of interest.

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Correspondence to Rob W. J. Collin PhD or Frans P. M. Cremers PhD.

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https://doi.org/10.1038/s41436-018-0414-9