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ISPD gene mutations are a common cause of congenital and limb-girdle muscular dystrophies

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Sebahattin Cirak, Aileen Reghan Foley, Ralf Herrmann, Tobias Willer, Shu Yau, Elizabeth Stevens, Silvia Torelli, Lina Brodd, Alisa Kamynina, Petr Vondracek, Helen Roper, Cheryl Longman, Rudolf Korinthenberg, Gianni Marrosu, Peter Nürnberg, , Daniel E. Michele, Vincent Plagnol, Matt Hurles, Steven A. Moore, Caroline A. Sewry, Kevin P. Campbell, Thomas Voit, Francesco Muntoni
DOI: http://dx.doi.org/10.1093/brain/aws312 269-281 First published online: 3 January 2013

Summary

Dystroglycanopathies are a clinically and genetically diverse group of recessively inherited conditions ranging from the most severe of the congenital muscular dystrophies, Walker–Warburg syndrome, to mild forms of adult-onset limb-girdle muscular dystrophy. Their hallmark is a reduction in the functional glycosylation of α-dystroglycan, which can be detected in muscle biopsies. An important part of this glycosylation is a unique O-mannosylation, essential for the interaction of α-dystroglycan with extracellular matrix proteins such as laminin-α2. Mutations in eight genes coding for proteins in the glycosylation pathway are responsible for ∼50% of dystroglycanopathy cases. Despite multiple efforts using traditional positional cloning, the causative genes for unsolved dystroglycanopathy cases have escaped discovery for several years. In a recent collaborative study, we discovered that loss-of-function recessive mutations in a novel gene, called isoprenoid synthase domain containing (ISPD), are a relatively common cause of Walker–Warburg syndrome. In this article, we report the involvement of the ISPD gene in milder dystroglycanopathy phenotypes ranging from congenital muscular dystrophy to limb-girdle muscular dystrophy and identified allelic ISPD variants in nine cases belonging to seven families. In two ambulant cases, there was evidence of structural brain involvement, whereas in seven, the clinical manifestation was restricted to a dystrophic skeletal muscle phenotype. Although the function of ISPD in mammals is not yet known, mutations in this gene clearly lead to a reduction in the functional glycosylation of α-dystroglycan, which not only causes the severe Walker–Warburg syndrome but is also a common cause of the milder forms of dystroglycanopathy.

  • congenital muscular dystrophy
  • limb-girdle muscular dystrophy
  • dystroglycan
  • laminin
  • isoprenoid synthase

Introduction

Congenital muscular dystrophies and limb-girdle muscular dystrophies (LGMDs) are characterized by hypotonia, muscle weakness, variable appearance of contractures and dystrophic changes on skeletal muscle biopsy. Although the congenital muscular dystrophies present either congenitally or during the first 6 months of life, the LGMDs present in late childhood, adolescence or adulthood (Voit, 1998; Bonnemann and Finkel, 2002). A number of genetically distinct entities have been identified within the congenital muscular dystrophies and LGMDs that are classified according to clinical and pathological criteria. An important subgroup, collectively known as the ‘dystroglycanopathies’, is associated with a reduction in the functional glycosylation of α-dystroglycan (Muntoni and Voit, 2004). Dystroglycan is composed of two subunits, α and β, which are post-translationally cleaved to give rise to a transmembrane (β) and external membrane protein (α), which is heavily O-glycosylated (Stalnaker et al., 2011). An important part of this glycosylation is a unique O-mannosylation sugar moiety that is involved in the interaction of α-dystroglycan with extracellular matrix proteins, such as laminin, agrin, perlecan, neurexin and pikachurin (Kanagawa and Toda, 2006; Waite et al., 2012). Mutations in eight genes coding for putative or demonstrated glycosyltransferases or other proteins involved in the α-dystroglycan glycosylation pathway have been identified in the dystroglycanopathies: protein O-mannosyltransferase 1 (POMT1; OMIM 607423) (Beltran-Valero de Bernabe et al., 2002), protein O-mannosyltransferase 2 (POMT2; OMIM 607439) (van Reeuwijk et al., 2005), protein O-mannose β-1, 2-N-acetylglucosaminyltransferase (POMGNT1; OMIM 606822) (Yoshida et al., 2001), fukutin (FKTN; OMIM 607440) (Kobayashi et al., 1998), fukutin-related protein (FKRP; OMIM 606596) (Brockington et al., 2001a), like-acetylglucosaminyltransferase (LARGE; OMIM 603590) (Longman et al., 2003) and dolichyl-phosphate mannosyltransferase polypeptide 3 (DPM3; OMIM 605951) (Lefeber et al., 2009). Recently, a missense mutation in the DPM3 gene was reported in a single patient with LGMD and stroke (Lefeber et al., 2009), and mutations in dolichol kinase (DOLK; OMIM 610746) have been reported in children with severe cardiomyopathy with reduced α-dystroglycan glycosylation and elevated serum creatine kinase levels (Lefeber et al., 2011). Interestingly, a single case was found to have a primary dystroglycanopathy due to a homozygous missense mutation at the N-terminus of dystroglycan 1 (DAG1; OMIM 128239) (Hara et al., 2011). The phenotypic spectrum arising from mutations in these dystroglycanopathy genes is extremely wide and includes (i) forms of congenital onset weakness and severe structural brain abnormalities, including Walker–Warburg syndrome (OMIM 236670; Walker, 1942; Warburg, 1971), muscle–eye–brain disease (OMIM 253280; Raitta et al., 1978) and Fukuyama congenital muscular dystrophy (OMIM 253800; Fukuyama, 1960); (ii) forms with congenital onset of weakness ranging from absent to severe brain involvement, including congenital muscular dystrophy type 1C (MDC1C; OMIM 606612) (Brockington et al., 2001a) and type 1D (MDC1D; OMIM 608840) (Longman et al., 2003); and (iii) forms with later-onset limb-girdle weakness associated with mental retardation and microcephaly but without structural brain defects as seen in LGMD type 2K (LGMD2K; OMIM 609308) (Dincer et al., 2003), and the mildest variants with no brain involvement, such as in LGMD type 2I (LGMD2I; OMIM 607155) (Brockington et al., 2001b). Mutations in these genes mentioned above are responsible for 50–60% of the cases classified as dystroglycanopathy (Godfrey et al., 2007; Mercuri et al., 2009; Messina et al., 2010; Devisme et al., 2012). Using traditional positional cloning, the causative genes for the unsolved dystroglycanopathy cases had escaped discovery. Cirak et al. (2009) mapped a novel disease locus to chromosome 7p21 in a family with loss of α-dystroglycan glycosylation.

Recently we discovered that bi-allelic loss-of-function mutations in the isoprenoid synthase domain containing (ISPD) gene, which maps to chromosome 7p21, are a frequent cause of Walker–Warburg syndrome (Willer et al., 2012). We now report the identification of nine patients from seven families who have mutations in ISPD, with phenotypes ranging from congenital muscular dystrophy to LGMD. These families included the original family mapped to 7p21 (Cirak et al., 2009). Here we present the clinical, genetic and pathological features of the milder phenotypic spectrum related to mutations in ISPD.

Materials and methods

Subjects and clinical assessments

The study was approved by the Institutional Ethical Review Board of the University College London Institute of Child Health and Great Ormond Street Hospital in the UK, the Ethical Review Board of the University of Duisburg-Essen in Germany and the Human Use Committee at the University of Iowa. Informed consent was obtained from the parents. The consent and local review board approval were in accordance with the UK10K project ethical framework (http://www.uk10k.org/ethics.html).

A three-generation family of Turkish origin with multiple loops of consanguinity demonstrating autosomal recessive inheritance was recruited (Supplementary Fig. 1). All three affected children and three unaffected siblings were examined, and serum creatine kinase levels were assessed in all siblings. The family was followed-up for >10 years, with the annual clinic visits at the University Children’s Hospital Essen in Germany.

Forty-seven patients with the clinical and pathological diagnosis of a dystroglycanopathy were recruited at the Dubowitz Neuromuscular Centre at the Great Ormond Street Hospital London, UK. Genomic DNA was extracted from blood using standard procedures. In all patients, mutations in POMT1, POMT2, POMGNT1, FKRP, FKTN and LARGE were excluded by Sanger sequencing. Of these 47 cases, 14 underwent initial exome sequencing, and an additional 33 were Sanger sequenced after the discovery of the ISPD gene mutations. Apart from the three cases of the Turkish family reported in this study, all other 44 cases were unrelated.

Histology and immunohistochemistry

Immunohistochemical studies were performed as described previously (Dubowitz and Sewry, 2007). Muscle biopsies were obtained using standard techniques and mounted in optimal cutting temperature medium, and were then frozen by immersion in isopentane cooled in liquid nitrogen. Unfixed, frozen serial sections (7 µm) were incubated with primary antibodies for 1 h at room temperature, followed by three washes in PBS. Sections were then incubated with anti-mouse– or anti-rabbit–biotinylated IgG or IgM-biotinylated secondary antibodies (General Electric Healthcare, 1:200) for 30 min at room temperature. After washing, muscle sections were incubated with streptavidin conjugated to Alexa Fluor® 594 (Invitrogen, 1:1000) for 15 min at room temperature, and then washed and mounted using Hydromount mounting medium (National Diagnostics). Primary antibodies used were mouse monoclonal: α-dystroglycan IIH6 (clone IIH6C4, 1:200), α-dystroglycan VIA4-1 (Merck Millipore, 1:50), β-dystroglycan (clone 43dag1/8d5, Leica, 1:20), laminin-α2 (MAB1922 clone 5H2 Merck Millipore, 1:4000) to the 80-kDa C-terminal fragment, laminin-γ1 (LT3 Merck Millipore, 1:4000), laminin-β2 (gift from Dr Ulla Wewer, Clone S5F11, 1:500) (Wewer et al., 1997) and β-spectrin (Leica, 1:20), rat monoclonal laminin-α2 (clone 4H8–2 Alexis Corporation, 1:100) N-terminal fragment, goat polyclonal core α-dystroglycan (GT20ADG, 1:20). Sections were evaluated using a Leica DMR microscope interfaced to MetaMorph (Molecular Devices). Muscle biopsies from Cases 1, 2, 8 and 9 were processed and reported in the diagnostic pathology units elsewhere. The muscle biopsy from Case 5 was evaluated according to the methods described by Willer et al. (2012).

Western blot and immunoblot

Western blot of the available muscle biopsy specimens was performed as described by Brockington et al. (2010). The following primary antibodies were used for the western blot of the muscle biopsies from Cases 4 and 7: anti-mouse α-dystroglycan IIH6 (Merck Millipore, catalogue 05-593), α-dystroglycan VIA4-1 (Leica, 1:50) and anti-mouse β-dystroglycan (Leica). Further experimental details are outlined in the Supplementary material. The muscle biopsy of Case 5 was studied using wheat germ agglutinin-enriched muscle homogenates as described previously (Michele et al., 2002). Immunoblots were done on polyvinylidene difluoride membranes as described earlier (Michele et al., 2002). The following antibodies were used for Case 5: the monoclonal antibodies to the fully glycosylated form of α-dystroglycan (IIH6 and VIA4) (Ervasti and Campbell, 1991) and α-dystroglycan (AP83) (Duclos et al., 1998). Shp5 (core-α-DG) from sheep antiserum was raised against the dystrophin–glycoprotein complex in its entirety and purified against a hypoglycosylated full-length α-DG–human IgGFc fusion protein (Kunz et al., 2001). Blots were developed by horseradish peroxidase enhanced chemiluminescence (Pierce).

Exome sequencing and data processing

Genomic DNA (1–3 μg) was sheared to 100–400 bp using a Covaris E210 or LE220 ultarsonicator. Sheared DNA was subjected to Illumina paired-end DNA library preparation and enriched for target sequences (Agilent Technologies; Human All Exon 50 Mb-ELID S02972011) according to the manufacturer’s recommendations (Agilent Technologies; SureSelectXT Automated Target Enrichment for Illumina Paired-End Multiplexed Sequencing). Enriched libraries were sequenced using the HiSeq platform (IIIumina) as paired-end 75-bp reads according to the manufacturer’s protocol. Sequencing reads that failed quality filtering were removed using the Illumina Genome Analyser Pipeline. The mean coverage of the exomes was 74 times with the descriptive exome, and statistical data are presented in Supplementary Table 1.

The Burrows–Wheeler Aligner (Li and Durbin, 2009) was used for alignment to the human reference genome build UCSC hg19, followed by the removal of polymerase chain reaction (PCR) duplicates using Picard (http://picard.sourceforge.net). The variant calling was performed in target ± 100-bp regions. For the variant calling, SAMtools (version 0.1.17) (Li et al., 2009) and Genome Analysis Toolkit (GATK)-Unified Genotyper (version 1.1-5) (McKenna et al., 2010) were used. Base quality recalibration and indel realignment were done with the help of GATK (DePristo et al., 2011). For each exome sample, variant sites (single nucleotide polymorphisms and indels) are called using the GATK-Unified Genotyper, and marked up with single nucleotide polymorphism database (dbSNP)132 rs-ids, GATK variant filtration applied (soft filter), including an indel mask consisting of 1000 Genomes pilot indels. Variants were assigned to quality tranches by GATK. The variants called by each of the callers were filtered separately using vcf-filter. For each sample, the resulting gatk.vcf and mpileup.vcf files were merged using vcf-isec. GATK annotations are preferred if sites are in both call sets. The variant calls were annotated using vcf-annotate for the following information: earliest version of dbSNP containing this call, dbSNP 132 rsIDs and 1000 Genomes population allele frequencies. The 1000 Genomes frequencies are taken from the June 2011 data release (http://www.1000genomes.org/data). Additionally, a number of functional scores were annotated to aid the filtering of variants. Further details of the variant calling and annotation procedures are listed in the Supplementary material.

Variant filtering

We used an in-house software to dynamically filter candidate variants on the basis of the autosomal recessive inheritance. Depending on the pedigree structure, we looked for either homozygous or two functional heterozygous changes in the same gene. The filtering at the ISPD locus was stringent, excluding the following variants: present in dbSNP132, present in 1000 Genomes, synonymous and other non-coding variants apart from essential splice site changes and not present in remaining UK10K rare disease cohort (322 exomes at the time of the analysis). None of the variants were present in the National Heart, Lung, and Blood Institute (NHLBI) Exome Sequencing Project database.

Copy number analysis

We used ExomeDepth (Plagnol et al., 2012, available at http://cran.r-project.org/) to fit a robust beta-binomial model to the read count data. By comparing read count between the test sample and additional exome samples from the same batch, this software predicts the expected read count. Deviations from this expectation are used to call copy number variants. ExomeDepth was run on all 14 cases who were whole-exome sequenced.

Experimental copy number validation

Quantitative fluorescent PCR analysis was performed as described previously (Yau et al., 1996). A single quantitative fluorescent PCR assay was designed to determine the copy number of exons 2, 3, 4, 5, 6, 7, 8, 9 and 10 of the ISPD gene by amplifying nine amplicons in a single 20-µl reaction using 6-FAM (Life Technologies) labelled forward primers and non-labelled reverse primers (primers and amplification conditions available on request). Fluorescent amplicons were analysed on an ABI 3730 DNA Analyzer (Applied Biosystems), and the data were then analysed with GeneMarker (SoftGenetics). The relative copy number of each exon was determined using dosage quotients as previously described (Yau et al., 1996).

Sanger sequencing

All exons and 50 bp of the flanking introns of the ISPD gene were sequenced from genomic DNA extracted from blood using standard protocols. PCR products were amplified using standard techniques and purified for sequence analysis with ExoI/shrimp alkaline phosphatase. Bi-directional fluorescent sequencing analysis was performed by the UCL genomic services using BigDye® v.1.1 Cycle Sequencing Kits (Applied Biosystems), which were analysed on an ABI 3730XL DNA Analyzer (Applied Biosystems) after purification using ethanol precipitation. Primer sequences are available on request. Each sequence was analysed visually using the Lasergene Seqman (DNASTAR) software.

Results

Clinical findings

We have identified nine cases from seven families with phenotypes milder than Walker–Warburg syndrome and ISPD mutations. Clinical features are summarized in Table 1, while a more detailed clinical case description is provided in the Supplementary material.

View this table:
Table 1

Clinical summary

CaseAge/sexPhenotype classificationSerum creatine kinase (IU/l)/ageAge of onset/ symptomsAge of maximal motor ability/ motor functionCurrent motor abilityPattern of muscle weaknessBrain MRIEye involvementOther features/age
121 years/FLGMD-no MR2000/1 month1.5 years/ frequent falls3–4 years/ managing stairsNon-ambulant since 12 yearsProximal, DMD-likeNormalNoCardiac: FS= 27%/19 years
214 years/FLGMD-no MR1800/14 months1.5 years/ Gowers’ sign3–4 years/ managing stairsNon-ambulant since 12 yearsProximal, DMD-likeNormalNoCardiac: mildly reduced LV function/12 years
34 years/FLGMD-no MR9097/4 years2 years/ Gowers’ sign4 years/ managing stairsFully ambulantProximal, DMD-likeNDNoNA
47 years/FCMD-no MR6000/16 months1 years/not standing5–6 years/ standing frameSittingProximalNDNoNA
511 years/FCMD/LGMD- no MR5000/1 years1 years/reduced movement in legs4–5 years/ managing stairsNon-ambulantProximalNormalNoNA
68.5 years/MLGMD-CRBa1500/6 months0.5 years/ oculomotor apraxia7 years/ runningFully ambulantProximalCerebellar cystsSevere myopia; oculomotor apraxiaNA
718 years/FLGMD-no MR4000/3.5 years3.5 years/ Gowers’ sign5 years/ managing stairsNon-ambulant since 12 yearsProximal, DMD-likeNormalNoCardiac: EF= 45%/18 years Respiratory: nocturnal hypoventilation/18 years
810 years/FLGMD-MR5849/6 years3 years/walking difficulties10 years/ runningFully ambulantProximalNormalNoCognitive: moderate learning difficulties
923 years/FLGMD-CRBa719/23 years0.5 years/severe myopia and strabismus5 years/ managing stairsStanding, few steps with assistanceProximalBrainstem hypoplasia; cerebellar hypoplasia; fourth ventricle dilatationSevere myopia; strabismusRespiratory: FVC= 49%/23 years Feeding: mild swallowing difficulties/23 years
  • a Newly proposed dystroglycanopathy category: limb-girdle muscular dystrophy with cerebellar involvement (LGMD-CRB).

  • CMD = congenital muscular dystrophy; DMD = Duchenne muscular dystrophy; EF = ejection fraction; FS = fractional shortening; FVC = forced vital capacity; LV = left ventricle; MR = mental retardation; NA = not applicable; ND = not done.

Cases 1, 2, 3, 5 and 7 have an LGMD-like phenotype without brain involvement (Fig. 1). Each of these five patients presented in early childhood with difficulty in walking and evidence of a Gowers’ sign. Case 3 is currently 4 years old and ambulant, but with proximal weakness and evidence of a Gowers’ sign. In Cases 1, 2, 3, 5 and 7, gross motor function improved until the age of ∼4 years, and all acquired the ability to climb stairs. Progression of proximal muscle weakness, however, led to loss of independent ambulation by the age of 12 years in Cases 1, 2 and 7. In Case 5 (Fig. 1), hypotonia was noted during the first year of life, but the subsequent disease course has been LGMD-like, making the overall phenotype intermediate congenital muscular dystrophy/LGMD-like. Generalized muscle hypertrophy was common, which included tongue hypertrophy in Cases 1 and 2 (Fig. 1). Case 8 is currently 10 years old and has a milder LGMD phenotype with learning difficulties. She is fully ambulant and can run slowly despite proximal muscle weakness. Case 4, currently aged 7 years, has a congenital muscular dystrophy phenotype without brain involvement. She never achieved independent walking or standing, but can use a self-propelling wheelchair and bottom shuffles.

In terms of cardiopulmonary involvement, a mild decrease in heart function with a fractional shortening of 27% was documented in Case 1 at the age of 19 years, for which isoprolol was started. The patient’s forced vital capacity was almost normal, at 85% predicted. Case 2 had mildly reduced left ventricular heart function noted at the age of 12, for which treatment with captopril was started. Case 7 developed nocturnal hypoventilation at the age of 18 years. Her ECG showed a reduced left ventricular ejection fraction of 45%. Case 9 developed respiratory insufficiency at the age of 23 years, with a forced vital capacity of 49% predicted. Her ECG revealed normal heart function.

Cases 6 and 9 (Fig. 1) have overlapping clinical features between congenital muscular dystrophy and LGMD and, for this reason, will be presented in more detail. Both presented in the first year of life with hypotonia and eye and brain involvement (with structural cerebellar and brainstem MRI abnormalities), but followed a relatively mild LGMD-like disease course. As their presenting symptoms were that of feeding and eye movement problems without weakness, this suggests that their early presentations were secondary to the CNS brain involvement, and not the severity of their muscle involvement. Case 6 is a boy aged 8.5 years. He presented at 6 months with a squint and was subsequently diagnosed with oculomotor apraxia, with difficulties in initiating saccades, a choroidal coloboma and severe myopia. Multiple cerebellar cysts were seen on brain MRI, and creatine kinase was >1500 IU/l. A muscle biopsy performed at 16 months identified a dystrophic process. From the developmental perspective, he sat with support at 8 months and started to walk at 15 months. At the age of 4 years, his head circumference was 50 cm (9th percentile), and he had evidence of axial weakness with subgravity neck and hip girdle power, but antigravity strength in the remaining muscles. He rose from the supine position with a Gowers’ sign. Ophthalmological examination revealed apraxic ocular movements and head thrusts, nystagmus at the extremes of gaze and an intermittent, alternating convergent squint. At his last clinical evaluation at the age of 7 years, he demonstrated further improvements. He stood with a lordotic posture and evidence of mild scapular winging. He rose from the floor in 1.4 s and had a waddling-type gait. Currently he is attending mainstream school with average academic achievements. Case 9 (Fig. 1) is a female who presented at birth with transient hypotonia and poor feeding. At 6 months of age, she was diagnosed with severe myopia and strabismus. She made rapid motor progress, and was able to sit at 6 months and walk at 18 months. At the age of 10 years, she lost the ability to rise from the floor. She is normocephalic. Her formal cognitive function was within the normal range (IQ of 89). At the age of 20, the examination showed paresis of superior oblique muscles and abducens muscles and strabismus without clear oculomotor apraxia. She also had myopia and buphthalmos. Currently, at 23 years of age, she can take a few steps indoors with assistance only and has been experiencing mild swallowing difficulties.

Figure 1

Clinical phenotype. Top: The clinical phenotype of ISPD-related muscular dystrophy in early childhood with pseudohypertrophy of lower limb muscles (A and B). Bottom: The disease at a later stage with marked pseudohypertrophy and ankle contractures (C, D and E). (A) Case 4 at 1.5 years, (B) Case 5 at 2.5 years, (C) Case 1 at 15.5 years, (D and E) Case 9 at 8 years.

Brain imaging

Brain imaging was available for Cases 1, 2, 5, 6, 7, 8 and 9. Brain magnetic resonance imaging (MRI) of Case 6 performed at 1 year showed multiple cerebellar cysts and supratentorial white matter changes (not shown). Case 9 had a brain MRI performed at 21 years that demonstrated brainstem hypoplasia, cerebellar hypoplasia, dilated fourth ventricle and evidence of bilateral buphthalmos (Fig. 3). The findings of the brain MRIs of the remaining cases were normal.

Muscle imaging

Muscle MRI was performed in Case 2 at 19.5 years and Case 9 at 20 years. Images revealed noticeable sparing of sartorius and gracilis muscles in both cases; sparing of the tibialis anterior muscle was more evident in Case 1 (Fig. 2). The degree of fibro-fatty replacement of muscle appeared to be concordant with the clinical severity.

Figure 2

Muscle MRI. (A) The T1-weighted muscle MRI of the thigh and calf of Case 1 at 19.5 years of age. (B) The T1-weighted muscle MRI of the thigh and calf of Case 9 at 20 years of age. There is sparing of sartorius and gracilis muscles (small arrows) in the thigh in both patients and sparing of the tibialis anterior muscle more visible in Case 1 (large arrow). The differential degree of fatty fibrous replacement is in concordance with the clinical severity with regards to ambulation, as Case 1 lost ambulation at 13 years, and Case 9 can still take a few steps with assistance only at age 23 years. AL = adductor longus; AM = adductor magnus; BF = biceps femoris; EDL = extensor digitorum longus; FDL = flexor digitorum longus; G = gracilis; GL = gastrocnemius lateralis; GM = gastrocnemius medialis; PG = peroneal group; RF = rectus femoris; S = sartorius; SM = semi-membranosus; SO = soleus; ST = semi-tendinosus; TA = tibialis anterior; TP = tibialis posterior; VL = vastus lateralis; VM = vastus medialis.

Figure 3

Brain MRI of Case 9 performed at 21 years of age, revealing brainstem hypoplasia, cerebellar hypoplasia and dilated fourth ventricle. (A) Sagittal T2-weighted image of the brain demonstrating brainstem hypoplasia, cerebellar hypoplasia and dilated fourth ventricle (arrow). (B) Axial T1-weighted image of the brain, revealing a normal appearance of the cerebral hemispheres. Interestingly, the temporalis muscles show some fibro-fatty changes (arrow). (C) Coronal T1-weighted image of the brain demonstrating dilatation of the fourth ventricle (arrow).

Muscle biopsy findings

Quadriceps muscle biopsies were performed in all cases except in Case 3. Routine histochemical studies revealed variable degrees of dystrophic features in all biopsies evaluated that included variation in fibre size, increased fibrosis and evidence of myonecrosis and regeneration. Immunolabelling with the α-dystroglycan antibodies (IIH6 and VIA4-1) was negative or severely reduced (Table 2). However, there was evidence of preserved expression of α-dystroglycan using the core antibody (GT20ADG) in those biopsies in which this analysis could be performed (Cases 4, 6 and 7) (Fig. 4). Laminin α-2 expression was reduced in all cases except in Case 5. Laminin α-2 immunolabelling was reduced in some cases (data not shown), whereas β-dystroglycan (Fig. 4) was generally well preserved (immunolabelling was slightly uneven on some fibres in Case 7, but no significant reduction was detected on immunoblots) (Supplementary Figs 5 and 6).

Figure 4

Immunohistochemistry of muscle biopsies from cases with ISPD-related muscular dystrophy. Unfixed frozen sections of quadriceps muscle biopsies from a control and three ISPD patients (Cases 4, 6, and 7) stained with haematoxylin and eosin (H & E) and immunolabelled with antibodies against laminin-α2 (LAMA2), β-dystroglycan (BDG), the glycosylated epitope of α-dystroglycan (IIH6 ADG) and the core protein of α-dystroglycan (GT20 ADG). Laminin-α2 immunostaining was reduced in all ISPD cases. Although expression of β-dystroglycan was similar to the control (see text), glycosylated α-dystroglycan immunolabelling was absent in Cases 4 and 7 and severely reduced in Case 6. Core α-DG (GT20ADG) was well preserved in all the cases.

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Table 2

Mutations and pathology

CaseaAge (years) at time of biopsyLaminin α-2α-dystroglycan (glycoepitope IIH6)α-dystroglycan (core 20)Genetic Screening techniquebVariant 1cVariant 2c
14Reduced on many fibresNegativeNDSangerExon 8: c.1114_1116del; p.(Val372del)Exon 8: c.1114_1116del; p.(Val372del)
21.5Reduced on many fibresNegativeNDSangerExon 8: c.1114_1116del; p.(Val372del)Exon 8: c.1114_1116del; p.(Val372del)
3FNDNDNDSangerExon 8: c.1114_1116del; p.(Val372del)Exon 8: c.1114_1116del; p.(Val372del)
42ReducedTracesMild reductionExomeExon 2: c.446C>T; p.(Pro149Leu)Exon 3: c.643C>T; p.(Gln215*)
51Positive (80-kDa epitope); slight reduction 300-kDa epitopeMany fibres negative (VIA4-1–traces)PositiveExomeExon 8: c.1114_1116del; p.(Val372del)Exon 9: Het c.1183A>T; p.(Arg395*)
61.3ReducedMany fibres negativeMild reductionExome/SangerExon 1: c.2T>G; p.(M1_R59del)Exon 2: c.377G>A; p.(Arg126His)
711Reduced on many fibresTracesPositive, mild reduction on some fibresExome/SangerExon 1: c.157G>A; p.(Ala53Thr)Exon 9: c.1183A>T; p.(Arg395*)
86Marked reduction on ImmunoblotTracesNDSangerExon 1: c.53dup; p.(Ser19Glufs*97)Exon 3: c.677A>G; p.(Tyr226Cys)
95NDNegativeNDExomeExon 6 to 8 duplication; c.836-?_1119+?dup; p.Val374Rfs*8Exon 6 to 8 duplication; c.836-?_1119+?dup; p.Val374Rfs*8
  • a Cases 1, 2 and 3 are affected individuals from the same family. Cases 4 to 9 are all unrelated individuals.

  • b Screening technique used to originally identify mutation: Exome = Next Generation Sequencing Exome; Sanger = dideoxy fluorescent sequencing; Exome/Sanger = indicate both techniques required to detect both mutations. Exon 1 of ISPD was not covered by the exome data and therefore additional Sanger sequencing of exon 1 was necessary.

  • c Mutation nomenclature follows the recommended guidelines (www.hgvs.orf/mutnomen) with the nucleotide numbering based on GenBank reference sequence NM_001101426.3. Nucleotide numbering denotes the adenosine of the annotated translation start codon as nucleotide position +1.

Immunoblot analysis

Because of sample availability, a western blot analysis was possible only in Cases 4, 5 and 7 (Supplementary Figs 5 and 6). The wheat germ agglutinin-enriched lysate from the muscle biopsy of Case 5 showed α-dystroglycan hypoglycosylation as suggested by the lack of binding affinity to the glycoepitope-specific antibodies IIH6 and VIA4-1. Western blot analysis of skeletal muscle of Cases 4 and 7 showed a profound reduction in α-dystroglycan expression using the IIH6 antibody, whereas β-dystroglycan expression was normal.

Genetics

All listed mutations are named according to reference sequence NM_001101426.3 (Fig. 5), corresponding to the long isoform of ISPD, which has 10 exons. Exon 3 of this long isoform is not present in the other short isoform (NM_001101417.3). Exome sequencing in Case 4 showed the following ISPD mutations at the heterozygous state: g.chr7: 16255759 T>A, c.446 C>T, causing p.Pro149Leu, which is located in exon 2 and g.chr7:16445774 G>A, c.643 C>T, p.Gln215* in exon 3. Exome sequencing in Case 5 showed a heterozygous premature stop codon mutation in exon 9: g.chr7:16255759 T>A, c.1183A>T, p.Arg395* and a heterozygous in-frame triplet deletion in exon 8: g.chr7:16298017 AAAC>A, c.1114-1116delGTT, leading to a single amino acid deletion p.Val372del. Exome sequencing in Case 6 showed a heterozygous missense mutation in exon 2: g.chr7:16445843 C>T, which is c.377G>A, leading to p.Arg126His. Interestingly, the second compound heterozygous mutation affecting the start codon in exon 1 c.2T>G, leading to p.M1_R59del or p.M1?, was identified only by Sanger sequencing, as exon 1 was not covered by the exome sequencing.

Figure 5

ISPD protein and mutations. The domain structure of the ISPD protein is illustrated and the corresponding exons are shown. The darker region represents the active functionally conserved CDP-ME domain (V47–A273). Mutations found in a compound heterozygous state are connected with a horizontal line. The small-sized horizontal bars represent the number of observed alleles. Bottom: The conservation of the missense mutations (marked with bold letters) within the vertebrates [Homo sapiens NP_001094896.1; Pan troglodytes (XP_003318374.1) 99% amino acid identity; Macaca mulatta (XP_001105001.2) 94% amino acid identity; Bos taurus (XP_002686725.1) 81% amino acid identity; Canis lupus familiaris (XP_003431914.1) 84% amino acid identity; Rattus norvegicus (NP_001008387.1) 73% amino acid identity; Mus musculus (NP_848744.1) 74% amino acid identity; Gallus gallus (XP_418693.2) 66% amino acid identity; Xenopus tropicalis (NP_001016240.1) 60% amino acid identity; Danio rerio (NP_001071270.1) 47% amino acid identity].

Exome sequencing in Case 7 revealed a heterozygous stop mutation in exon 9: g.chr7:16255759 T>A, leading to c.1183 A>T and causing p.Arg395*. The second compound heterozygous mutation was found by Sanger sequencing to be c.157G>A causing p.Ala53Thr located in exon 1. All ISPD mutations found by exome sequencing were confirmed by Sanger sequencing.

Following the discovery of mutations in the ISPD gene by whole exome sequencing, the original family that was mapped to chromosome 7p21 was screened for mutations in all 10 exons of the ISPD gene by Sanger sequencing. All the affected individuals in this family (Cases 1, 2 and 3) were found to have inherited a homozygous 3-bp deletion in exon 8 resulting in a single amino acid deletion (c.1114-1116delGTT; p.Val372del). The mutation was found to be co-segregating with the phenotype. In the remaining cases, we identified one patient (Case 8) with a frameshift mutation (c.53dupT) in exon 1 and a missense mutation in exon 3 c.677A>G (p.Tyr226Cys). The heterozygous carrier status of the parents demonstrating the expected phase for an autosomal recessive inheritance was confirmed in all families except in the family of Case 6, as parental DNA was not available.

A read depth copy number analysis (R package ExomeDepth, Plagnol et al., 2012) of the exome sequence from Case 9 detected double the number of expected reads in a 40 916 kb region [chr7:16276936–16317852 (UCSC hg19)] involving exons 6, 7 and 8 of the ISPD gene (Supplementary Fig. 2). Quantitative fluorescent PCR analysis of genomic DNA confirmed that ISPD exons 6, 7 and 8 were homozygously duplicated in Case 9, resulting in an out-of-frame duplication (Supplementary Fig. 4) and that both her parents were carriers of the mutation (data not shown).

Discussion

Functional glycosylation defects of α-dystroglycan represent a major pathological subgroup of congenital and LGMDs. These so-called dystroglycanopathies range from a lethal clinical variant of Walker–Warburg syndrome with cerebral and ocular involvement to milder forms of adult-onset LGMD such as LGMD2I (Godfrey et al., 2007). Although each of the eight known genes that code for putative or demonstrated glycosyltransferases or proteins involved in the glycosylation of α-dystroglycan could in theory cause each of these clinical variants, there has been a marked difference in frequency and clustering of phenotypes for certain known genes so far. Mutations in FKRP are the most common cause of dystroglycanopathy in the UK (Mercuri et al., 2003, 2009; Poppe et al., 2003) and can cause the entire spectrum of dystroglycanopathy phenotypes (Brockington et al., 2002; Brown and Winder, 2012; Devisme et al., 2012). Other genes such as POMGNT1, POMT1 and POMT2 are mostly responsible for phenotypes with CNS involvement (Mercuri et al., 2009; Messina et al., 2010; Brown and Winder, 2012; Devisme et al., 2012). The DPM3 and DOLK genes, which represent an overlapping group with N-glycosylation disorders and dystroglycanopathies, are rare, as only a handful of cases have been described to date (Lefeber et al., 2009, 2011; Brown and Winder, 2012). The genetic aetiology of this group is indeed diverse, and ∼50% of the cases with dystroglycanopathy remain unsolved (Wewer et al., 1997; Mercuri et al., 2009). After the discovery of bi-allelic loss-of-function mutations in ISPD causing Walker–Warburg syndrome (Roscioli et al., 2012; Willer et al., 2012), we can now describe the full spectrum of phenotypes caused by recessive mutations in ISPD including a quite common milder allelic LGMD phenotype. The spectrum of the phenotypes ascertained in this study ranges from cases with congenital muscular dystrophy without CNS involvement (Case 4), milder cases with LGMD without CNS involvement (Cases 1, 2, 3, 5 and 7) (Fig. 1) and a rather unusual and novel phenotype with relatively mild skeletal muscle weakness manifesting as a LGMD and structural brain involvement affecting predominantly the subtentorial structures (Cases 6 and 9) (Fig. 1), confirming once again the preferential involvement of subtentorial structures in dystroglycanopathies (Clement et al., 2008). This phenotype is in contrast to LGMD2K, which is associated with microcephaly and mental retardation (Lommel et al., 2010), a phenotype that Case 8 in our series resembles. As an LGMD phenotype with structural cerebellar involvement has not been reported in any of the remaining dystroglycanopathies, this combination of features appears to be highly evocative of an ISPD-related muscular dystrophy. We suggest the use of the term ‘limb-girdle muscular dystrophy with cerebellar involvement’ (LGMD-CRB) to describe these patients. This term could be added to the recently proposed classification of dystroglycanopathies (Godfrey et al., 2011).

As in other dystroglycanopathies, ISPD-related disease is progressive, with most cases with LGMD losing ambulation in their early teenage years, thus following a Duchenne muscular dystrophy-like path. In several patients, there was muscle pseudohypertrophy, including the tongue. Respiratory and cardiac functions also demonstrated decline, resembling that reported for other dystroglycanopathies (Mercuri et al., 2003; Murakami et al., 2006; Bourteel et al., 2009; Lefeber et al., 2011; Yilmaz et al., 2011). Therefore, regular surveillance of heart function by ECG and respiratory function by regular overnight polysomnography is required in ISPD-related muscular dystrophy. Muscle MRI shows replacement with fat and connective tissue in the lower limbs with sparing of the semitendinosus and gracilis muscles in the thighs and the tibialis anterior muscle in the calves. Interestingly, the gracilis muscle is also spared in FKRP-related LGMD2I (Bourteel et al., 2009).

From the histopathological perspective, all cases show substantially reduced IIH6 or VIA4-1 labelling, indicating the loss of functional α-dystroglycan glycosylation. Using immunocytochemistry, there were no clear differences in IIH6 staining between severe and milder phenotypes in the majority of cases. The lack of correlation between severity of skeletal muscle involvement and loss of the IIH6 epitope on immunocytochemistry and immunoblot (even after wheat germ agglutinin enrichment, Case 5) is quite striking in ISPD-related muscular dystrophy. Variable correlations between clinical phenotype and IIH6 content in skeletal muscle have been reported for mutations in other genes such as FKRP and FKTN (Jimenez-Mallebrera et al., 2009), while there appears to be a better correlation for POMT1-, POMT2- and POMGNT1-related dystroglycanopathies (Jimenez-Mallebrera et al., 2009; Lommel et al., 2010). This poor correlation (i.e. apparent severe depletion of IIH6 epitope also in patients with relatively milder variants) may be due to the fact that there is some laminin-binding activity on α-dystroglycan owing to other glycans that are not recognized by IIH6 (McDearmon et al., 1998, 2001, 2003, 2006; Stalnaker et al., 2010, 2011). Our genetic data (Fig. 5) demonstrate a good genotype–phenotype correlation in the ISPD-related muscular dystrophy. We have previously shown (Willer et al., 2012) that bi-allelic loss-of-function mutations cause a Walker–Warburg syndrome phenotype. Compound heterozygosity of a missense mutation and a loss-of-function mutation affecting one of the first five exons of ISPD results in a congenital muscular dystrophy phenotype (Case 4), LGMD-CRB phenotype (Case 6) or a LGMD phenotype with mental retardation (Case 8), because the first five exons of ISPD contain the functional conserved 4-diphosphocytidyl-2-methyl-D-erythritol synthase (CDP-ME) domain. The cases with milder LGMD without brain involvement have either a homozygous in-frame deletion of a single amino acid in exon 9 (p.V372del) (Cases 1, 2 and 3) or are compound heterozygous for a mild mutation and a stop mutation in exon 9 (Cases 5 and 7). Mutations in other domains could also alter the function of ISPD substantially, as a homozygous stop mutation p.Glu396* has been reported to cause a Walker–Warburg syndrome phenotype (Roscioli et al., 2012). The effect of the homozygous duplication of exons 6, 7 and 8 in Case 9 is also interesting. We predicted that the open reading frame would be translated until exon 8 and followed by a frameshift in exon 9, which could lead to a truncated ISPD protein (Val374Rfs*8). The mild phenotype in this patient is surprising and could be accounted for by a number of different mechanisms: (i) there could be a splicing aberration leading to the production of reduced levels of an in-frame message; (ii) the truncated protein could be partly active, as the CDP-ME containing exons of ISPD are translated; and (iii) there could be incomplete nonsense-mediated decay related to the mutation occurring towards the 3′ end of the gene. The question that remains is how these dystroglycanopathy phenotypes might be explained by the putative function of ISPD. In eubacteria, green algae and chloroplasts of higher plants, ISPD orthologues are part of the methylerythritol pathway. This pathway contains the CDP-ME domain and catalyzes the third step in the alternative (non-mevalonate) pathway of isopentenyl diphosphate biosynthesis (isoprenoid precursor). The formation of 4-diphosphocytidyl-2C-methyl-d-erythritol from cytidine triphosphate and 2C-methyl-d-erythritol 4-phosphate is also called cytidyltransferase activity. This mevalonate-independent pathway uses pyruvate and glyceraldehyde 3-phosphate as starting materials for production of isopentenyl diphosphate and occurs in a variety of bacteria, archaea and plant cells but is absent in mammals, which suggests that ISPD must have a different function(s) in humans. The mechanism by which ISPD mutations lead to a reduction of α-dystroglycan glycosylation is not well understood. Apart from the CDP-ME domain, ISPD also contains and belongs to the glycosyltransferase-A family (Breton et al., 2006). Interestingly, LARGE also belongs to this glycosyltransferase-A family. The function of LARGE has been partly elucidated; it acts as a bi-functional glycosyltransferase, with both xylosyltransferase and glucuronyltransferase activities, attaching repeating units of [-3-xylose-α1,3-glucuronic acid-β1-] to α-dystroglycan (Inamori et al., 2012). Considering that there are also some prokaryotes that lack the methylerythritol pathway and contain homologous enzymes such as TarI in Streptococcus pneumonia, which synthesizes activated CDP-ribitol (Baur et al., 2009; Roscioli et al., 2012), one could hypothesize that in vertebrates ISPD activates nucleotide sugar building blocks for complex α-dystroglycan glycosylation or even that it could have complex glycosyltransferase activity similar to LARGE. However, the experimental evidence reported in our recent study (Willer et al., 2012) suggests that in patients with ISPD-deficient Walker–Warburg syndrome, O-mannosylation was strongly impaired and subsequently the O-mannosyl phosphorylation and LARGE-dependent hyperglycosylation were absent (Willer et al., 2012). This indicates the pivotal role for ISPD in the initial step of the O-mannosylation of α-dystroglycan.

Mutations in ISPD appear to be relatively common; in our previous population study (Willer et al., 2012), we evaluated 92 patients with dystroglycanopathy after exclusion of FKRP, and the most frequent mutations found were in POMT1 and POMT2 (8.6% each). Here we have screened 47 cases, and 7 of 44 (16%) non-familial cases have mutations in ISPD. We recently reported that 30% of the Walker–Warburg syndrome cohort and 11% of the dystroglycanopathy cohort (Willer et al., 2012) have ISPD mutations, similar to another report on Walker–Warburg syndrome (Roscioli et al., 2012). The ISPD gene also appears to be frequently affected by copy number variations (Willer et al., 2012); therefore, testing for copy number variations in ISPD will be essential in the diagnostic evaluation of patients with dystroglycanopathy.

In conclusion, ISPD mutations are a common cause of secondary dystroglycanopathy with a phenotypic spectrum ranging from Walker–Warburg syndrome to LGMD. As the laminin-binding glycoepitope is almost undetectable in most of the cases with ISPD-related muscular dystrophy, the elusive function of ISPD must have a pivotal role for functional α-dystroglycan glycosylation. Uncovering of the ISPD function will help to decipher the glycosylation pathway of α-dystroglycan.

Funding

The authors are grateful to the Wellcome Trust funded UK10K consortium for making this study possible. A.R.F. is a Muscular Dystrophy Campaign Fellow. F.M. is supported by the Great Ormond Street Children’s Charity and the GOSH Biomedical Research Centre. This study was supported by the Muscular Dystrophy Campaign grant on congenital muscular dystrophy, the MRC Neuromuscular Centre Biobank, Great Ormond Street Hospital Charity and European BIO-NMD FP7 consortium. The National Specialised Commissioning Team (NSCT) funding for the Congenital Muscular Dystrophies and Congenital Myopathy service in London is gratefully acknowledged. Iowa Wellstone Muscular Dystrophy Cooperative Research Center, U54, NS053672, National Institute of Neurological Disorders and Stroke for T.W., S.A.M., K.P.C. and F.M.. K.P. Campbell is an investigator of the Howard Hughes Medical Institute.

Supplementary material

Supplementary material is available at Brain online.

Web resources

The Variant Call Format and VCFtools, Petr Danecek, Adam Auton, Goncalo Abecasis, Cornelis A. Albers, Eric Banks, Mark A. DePristo, Robert Handsaker, Gerton Lunter, Gabor Marth, Stephen T. Sherry, Gilean McVean, Richard Durbin and 1000 Genomes Project Analysis Group, Bioinformatics, 2011, http://vcftools.sourceforge.net/; Tennessen JA, Bigham AW, O'Connor TD, Fu W, Kenny EE, Gravel S, McGee S, Do R, Liu X, Jun G, Kang HM, Jordan D, Leal SM, Gabriel S, Rieder MJ, Abecasis G, Altshuler D, Nickerson DA, Boerwinkle E, Sunyaev S, Bustamante CD, Bamshad MJ, Akey JM; Broad GO; Seattle GO; NHLBI Exome Sequencing Project. Evolution and functional impact of rare coding variation from deep sequencing of human exomes. Science. 2012 Jul 6;337(6090):64-9. Epub 2012 May 17. PubMed PMID: 22604720. http://evs.gs.washington.edu/EVS/

Acknowledgements

The authors thank Dr Lucy Feng and Darren Chambers for the excellent processing of muscle biopsy specimen and muscle biopsy images. They thank Prof Knut Brockmann, Dr Lars Klinge, Dr Adnan Manzur and Dr Stephanie Robb for providing clinical information, and Dr Emma Clement and Dr Caroline Godfrey for their earlier work on the dystroglycanopathy cohort. The NSCT Newcastle Biopsy Service is also acknowledged for providing the pathology report of Case 8.

Footnotes

Abbreviations
CDP-ME
4-diphosphocytidyl-2-methyl-D-erythritol synthase
LGMD
limb-girdle muscular dystrophy

This is an Open Access article distributed under the terms of the Creative Commons Attribution Non-Commercial License (http://creativecommons.org/licenses/by-nc/3.0/), which permits unrestricted non-commercial use, distribution, and reproduction in any medium, provided the original work is properly cited.

References

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