- Open Access
A novel mechanism for variable phenotypic expressivity in Mendelian diseases uncovered by an AU-rich element (ARE)-creating mutation
- Nisha Patel1,
- Arif O. Khan1, 2,
- Maher Al-Saif3,
- Walid N. Moghrabi3,
- Balsam M. AlMaarik1,
- Niema Ibrahim1,
- Firdous Abdulwahab1,
- Mais Hashem1,
- Tarfa Alshidi1,
- Eman Alobeid1,
- Rana A. Alomar1,
- Saad Al-Harbi4,
- Mohamed Abouelhoda1, 6,
- Khalid S. A. Khabar3Email author and
- Fowzan S. Alkuraya1, 5, 6Email author
© The Author(s). 2017
- Received: 13 April 2017
- Accepted: 6 July 2017
- Published: 28 July 2017
Variable expressivity is a well-known phenomenon in which patients with mutations in one gene display varying degrees of clinical severity, potentially displaying only subsets of the clinical manifestations associated with the multisystem disorder linked to the gene. This remains an incompletely understood phenomenon with proposed mechanisms ranging from allele-specific to stochastic.
We report three consanguineous families in which an isolated ocular phenotype is linked to a novel 3′ UTR mutation in SLC4A4, a gene known to be mutated in a syndromic form of intellectual disability with renal and ocular involvement. Although SLC4A4 is normally devoid of AU-rich elements (AREs), a 3′ UTR motif that mediates post-transcriptional control of a subset of genes, the mutation we describe creates a functional ARE. We observe a marked reduction in the transcript level of SLC4A4 in patient cells. Experimental confirmation of the ARE-creating mutation is shown using a post-transcriptional reporter system that reveals consistent reduction in the mRNA-half life and reporter activity. Moreover, the neo-ARE binds and responds to the zinc finger protein ZFP36/TTP, an ARE-mRNA decay-promoting protein.
This novel mutational mechanism for a Mendelian disease expands the potential mechanisms that underlie variable phenotypic expressivity in humans to also include 3′ UTR mutations with tissue-specific pathology.
- AU-rich elements
- Variable expressivity
All the cells of an individual share an identical genome, barring postzygotic mutations, yet they display strikingly different structural and functional characteristics attributed to diverse transcriptional profiles . This basic concept is frequently invoked to explain the selective involvement of a subset of organs in diseases caused by germline mutations, i.e. only tissues that express the mutated gene are subject to the pathological effect of mutations therein. However, the observation that in many pleiotropic diseases, the multisystem involvement is highly variable among patients (also known as variable expressivity), poses a challenge to this concept since the gene is clearly both expressed and required by the tissues that are only affected in some patients but not others . Variable expressivity is one of the most challenging obstacles in variant interpretation and understanding its underlying mechanism, therefore, can have a significant impact on the delivery of genomic medicine.
Several mechanisms have been proposed to explain variable expressivity and they need not be mutually exclusive . For example, Bardet–Biedl syndrome is a multisystem ciliopathy and yet several mutations have been reported to cause an eye-limited phenotype. At least in one such instance, it has been shown that the eye-specific mutation affects an eye-specific transcript, consistent with the identification of tissue-specific exons [4, 5]. Allele-specific variable phenotypic expressivity can also uncover a tissue-variable threshold where tissues display different susceptibility depending on the level of gene deficiency. For example, mild mutations in the gene encoding phosphoglycerate dehydrogenase cause a brain-specific phenotype whereas more severe deficiency causes a lethal multisystem disease known as Neu-Laxova syndrome [6, 7]. Alternatively, coding mutations may cause a pleiotropic phenotype whereas enhancer mutations will only affect the tissues in which that enhancer is active, as observed in PTF1A-related cerebellar and pancreatic agenesis versus PTF1A-related isolated pancreatic agenesis [8, 9]. However, this genotype/phenotype correlation is often lacking and variable expressivity can be seen in the context of the same mutation. Proposed mechanisms in such instances include variable splicing efficiency (e.g. TCTN1-related ciliopathies), the requirement for postzygotic second mutations (e.g. neurofibromatosis), or other genetic modifiers, as well as stochastic events [10, 11]. Clearly, much remains to be understood about the factors that control this phenomenon.
Mutations in the untranslated region (UTR) of genes are extremely rare causes of Mendelian diseases and even the few described (e.g. FMR1-related fragile-X syndrome, DMPK-related myotonic dystrophy) tend to represent repeat expansion. While 5′UTR point mutations causing Mendelian diseases have rarely been described, 3′UTR mutations in the context of Mendelian phenotypes are even rarer [12–15]. A few of these examples include a compound heterozygous mutation in GFPT1, which includes a 3′UTR mutation (c.*22C > A) has been reported to cause congenital myasthenic syndromes by the formation of a microRNA target site . Additionally, 3′UTR mutation in FMR1 has been shown to cause fragile X syndrome by disrupting the mRNA binding protein HuR, leading to destabilization and rapid degradation of the FMR1 transcript . Interestingly, both 5′UTR and 3′UTR mutations in GJB1 have been reported to cause Charcot–Marie–Tooth disease . In the context of multifactorial diseases, however, several 3′UTR SNPs have been reported with suggested influence on disease susceptibility . These include rs356165 in SNCA encoding alpha-synuclein as a potential susceptibility locus for Parkinson disease , rs3027898 in IRAK1 as a potential susceptibility locus for rheumatoid arthritis , and another 3′UTR SNP in hPTP1B associates with insulin resistance . In this study, we describe, to our knowledge, the first ARE-creating mutation in the context of a Mendelian phenotype and propose a novel allele-specific mechanism for variable expressivity as a result.
Patients were evaluated clinically followed by enrollment in an IRB-approved research protocol with informed consent (KFSRHC RAC# 2070023). Parents and available siblings were also recruited. Venous blood was collected from all participants in EDTA tubes and, in a subset of patients, in sodium heparin tubes for DNA extraction and establishment of lymphoblastoid cell lines (LCL), respectively.
Autozygosity mapping and exome sequencing
DNA samples from all available family members were genotyped on the Axiom SNP chip platform following the manufacturer’s instructions, followed by autozygome analysis using AutoSNPa . Runs of homozygosity that are > 2 Mb in length were considered as surrogates of autozygosity given the consanguineous nature of the families and the overlapping autozygome between the affected individuals only was considered as a candidate positional locus as described before [24, 25]. For exome analysis, we selected the index from two families. The samples were prepared according to the preparation guide of Agilent SureSelect Target Enrichment Kit and the resulting libraries were sequenced using the Illumina HiSeq2000 sequencer. The Genome Analysis Toolkit (GATK) was used for variant calling.
mRNA level assays
In the two human participants for which LCL were established, RNA was extracted from cell pellets followed by relative quantification of the SLC4A4 (MIM#604278). Total RNA from patients and control lymphoblast cell lines were extracted using QIAamp RNA mini Kit (Qiagen inc., Germantown, MD, USA) with DNAase treatment (Qiagen), according to manufacturer’s instructions. cDNA was prepared using the iScript™ cDNA synthesis kit and poly-T oligonucleotide primers (Applied Biosystems, Carlsbad, CA, USA). Relative quantification reverse transcription polymerase chain reaction (RT-QPCR) was performed using SYBR green and Applied Biosystems 7500 Fast Real-Time PCR system. Primers were designed to flank an intron to specifically amplify cDNA (SLC4A4 5’- ATTCCTTGAACGCCACACAT; 5’- TTTCTGTTCCCTTGCTCCTC), generating 159 bp amplicon. Melt curve analysis was performed to confirm that a single product was amplified. Gene expression was normalized to GAPDH and all reactions were run in triplicate and repeated as three independent experiments.
HeLa epithelial cells, human kidney HEK293 cell line, neuroblastoma NB-A, and normal human fibroblasts were obtained from the American Type Culture Collection (ATCC; Rockville, MD, USA). The HAP-1 wild-type (WT) and CRISPR ZFP36-knockout haploid fibroblast –like cell line were obtained from Horizon Discovery (UK) and cultured in Iscove’s Modified Dulbecco’s Medium with 10% fetal bovine serum (FBS) and 1% antibiotics. HeLa and HEK cell lines were maintained in Dulbecco’s modified Eagle’s medium (DMEM), while neutroblastoma and fibroblasts were maintained in MEM (ThermoFisher, Carlsbad, CA, USA) supplemented with 10% (FBS) and antibiotics. Tet-On and Tet-Off Advanced HeLa cells were obtained from ClonTech and were maintained in DMEM supplemented with 10% Tet-System Approved FBS (ClonTech) and antibiotics and maintained in selection medium (100 μg/mL G418; Sigma).
Cloning of ARE reporter constructs
The RPS30 promoter (RPS30)-linked reporter expression vectors  containing a 70-base region from the normal control SCL4A4 3′UTR and the ARE-creating mutant 3′UTR were constructed using synthetic oligos. The oligo sequence is: TGTCATTTGTTTTTGTTTGGCTGTTTGTTTATTTTTTAACTTTTATTTCGTCTCAGTTT TTGG, where G to A is in the oligo with the ARE-creating mutant. The oligonucleotides were designed to contain (G/GATCC) BamHI and (T/CTAGA) XbaI overhangs. The annealed oligos were cloned in BamH1 and XBaI sites in the 3′UTR of the RPS30-nanoluciferase vector. The use of the transcriptionally non-inducible RPS30 promoter allows selective post-transcriptional effects.
Transfection and reporter activity measurements
Cells were plated at 2 × 105 cells/mL per well in 96-well plate overnight and co-transfected with RPS30 promoter-linked nanoluciferase fused with the 3′UTR containing WT and mutant sequences along with firefly luciferase vector as a normalization control. The cells were transfected using Lipofectamine 2000 (Invitrogen) according to the manufacturer’s instructions. Transfections were performed in several replicates. After 16 h, cells were lysed and assayed for luciferase activity using the dual Nano-Glo dual-luciferase assay kit (Promega) according to the manufacturer’s instructions and measured on a luciferase luminometer. Data were presented as mean ± SEM of normalized Nano luciferase intensity/firefly intensity.
mRNA half-life experiments
For actinomycin D chase-based mRNA half-life determination, actinomycin D (5 μg/mL; Sigma) was used to block transcription. For Tet-off based determination of mRNA half-life, the reporter constructs were converted to Tet-regulated cassettes by inserting multiple copies of TetO sites in a minimal cytomegalovirus (CMV) promoter, as previously described . The Tet-off reporters fused with the WT or mutant 3′UTR were transfected to HeLa Tet-off cells overnight and then treated with doxycycline (0.25 μg/mL) to shut off transcription for 1, 2, 4, 6, and 24 h.
The RNA was extracted by Trizol at multiple points following transcriptional shut off and then subjected to RT-QPCR. The RT reaction was performed using total RNA, 150 ng random primers, 10 mM dNTP mixture, 40 U/μL RNase inhibitor, and 200 units of SuperScript II RT. RT-QPCR was performed as multiplex reactions in a CFX96 cycler (Bio-Rad, Hercules, CA, USA) using FAM-labeled TaqMan probe/primers for Nanoluciferase: the nanoluciferase primer/probes were custom-synthesized by Metabion: (forward primer: 5′-CTCCATCTTCGCGGTAGCT -3′, reverse primer: 5′-GAGGACTTGGTCCAGGTTGTA -3′, and FAM-labeled TaqMan probe: 5′-Fam-CCGCCGTTCAGTCGCCGT -BHQ-1-3′). The RNA samples were normalized with VIC-labeled ribosomal protein (PO) probe. Samples were amplified in triplicate and quantification of relative expression was performed using the ΔΔCt method. The mRNA half-life was calculated using the one-phase exponential decay method (GraphPad Software, San Diego, CA, USA). The equation Y = Span × exp(–K × X) + Plateau describes the kinetics of mRNA decay. X is time and Y represents the response. SPAN and PLATEAU are expressed in the same units as the Y axis. K is expressed in the inverse of the units used by the X axis. Y starts as equal to SPAN + PLATEAU and decreases to PLATEAU with a rate constant K. The mRNA half-life of the decay is 0.6932/K. This method has the best fit for mRNA data that tend to decay at a certain rate over a period of time and then reach a plateau. Using the least squares fit method, the fits were > R = 0.9.
RNA immunoprecipitation and immunoblotting
HEK-293 cells were transfected overnight with 500 ng vector expressing HA-tagged ZFP36 (previously known as TTP). Cells were lysed in RNA immunoprecipitation (RNA-IP) buffer consisting of 0.5% NP40, 100 mM KCl, 10 mM HEPES (pH 7.0), 5 mM MgCl2, freshly supplemented before use with 1 mM DTT, 5 μL/mL units RNase Out (ThermoFisher), and protease inhibitor mix (Roche). The lysates were centrifuged at 12,000 rpm and the supernatants obtained were incubated with monoclonal anti-HA antibody (for ZFP36) or monoclonal anti-Myc antibody as background control (coupled with pre-swollen protein G-sepharose beads). Aliquots were collected for western blotting and the remaining beads were used for RNA extraction using RNazol (Sigma), followed by chloroform and isopropanol precipitation. The cDNA was synthesized using SuperScript II RT (ThermoFisher). RT-QPCR was performed in multiplex reaction in a thermal cycler (Bio-Rad) using the nanoluciferase and PO primer/probe combination.
To confirm transfection and expression of the ZFP36, total lysates were subjected to western blotting using anti-HA antibody while anti-Myc antibody was used as a negative control as previously described . Signal detection was performed with ECL western blotting detection reagents (Amersham Biosciences, UK). Protein molecular weight markers were used to verify the protein size.
Functional response of the SLC4A4 neo-ARE towards ZFP36
Tetracycline inducible (Tet-On) ZFP36 expressing cassettes were constructed by PCR of pCR3.1-ZFP36 plasmids using the forward primer that includes multiple copies of the TetO site as previously described . HeLa Tet-On Advanced cells were transfected with 50 ng of either the WT or mutant 3′UTR fused-nanoluiferase reporters along with Firefly plasmid normalization control and 10 ng of the TetO-ZFP36 constructs. Transfections were performed using Lipofectinamine 2000 (Invitrogen) according to the manufacturer’s instructions. Doxycycline (0.25 ug/mL) was added to the transfected cells for 16 h and luminescence was acquired by luminometer. Data were presented as mean ± SEM of normalized Nano luciferase intensity/firefly intensity.
Isolated keratopathy is caused by a 3′UTR variant in SLC4A4
Isolated band keratopathy mutation creates an AU-rich element
Neo-ARE in SLC4A4 induces post-transcriptional effects in gene expression
The neo-ARE introduced in the patient’s SLC4A4 gene with isolated ocular phenotype belongs to canonical class I ARE that harbors UUAUUUAUU in U-rich context. We first introduced the AU-rich region that contains the *206G>A mutation or the WT sequence with their flanking region in the 3′UTR of a post-transcriptional reporter vector (Fig. 3a) . This selective post-transcriptional assessment system has been established with non-transcriptional inducible promoter (RPS30) and UU/UA reduced reporter coding region [26, 31]. We compared the mutant with WT 3′UTR constructs and found a consistent and appreciable reduction in the activity of the reporter fused to the ARE-forming (mutant) 3′UTR (Fig. 3b). This effect was observed in multiple different cell lines representing both of epithelial and fibroblast tissues. Specifically, there was a significant reduction (26–57%, P < 0.0001) depending on the cell line used (Fig. 3b).
The SCL4A4 neo-ARE physically associates and responds to ZFP36
AU-rich elements are among the most important regulatory elements that post-transcriptionally control the expression of many genes in mammalian cells. AREs are characterized by the presence of consensus pentamer AUUUA in U-rich context such as the nonamer UUAUUUA(U/A)(U/A) and they can exist in clusters of two to six [32, 33]. AREs are enriched in transiently expressed genes in which they play a key role in their tight temporal regulation. This control is mediated by trans-acting factors in the form of RNA-binding proteins as well as microRNAs; such effects are not limited to RNA stability regulation but also translational efficiency .
Despite the established role of AREs, most of the knowledge about its role in human diseases is in the context of complex diseases such as cancer rather than Mendelian diseases . Indeed, we are not aware of variants creating a typical ARE (Class I or Class II) in the context of any human disease. In the families we present, we show that an isolated ocular phenotype in the form of band keratopathy with or without congenital glaucoma is linked to a novel variant that creates a neo-ARE in a gene that normally lacks it. Our data strongly suggest that this neo-ARE induces ZFP36-mediated effect on the post-transcriptional control of SCL4A4. The consistent lack of any syndromic feature in all patients with this mutation is in striking contrast to the known syndromic phenotype associated with coding mutations in SLC4A4, i.e. severe renal and ocular involvement with intellectual disability . This suggests that the destabilization of SLC4A4 mRNA was only severe enough to induce the ocular sub-phenotype of an otherwise multisystem syndrome.
Coding versus enhancer mutations are well-known to explain some instances of variable expressivity. For example, coding mutations in SOX9 are established causes of the lethal disorder campomelic dysplasia. However, point mutations in the craniofacial-specific enhancer cause a much-limited Pierre-Robin phenotype . Our finding that the creation of a neo-ARE with a tissue-specific pathological consequence, therefore, suggests a novel biological aspect of ARE that has potentially important implications for the phenomenon of variable expressivity akin to that of coding versus enhancer mutations. Enhancer elements are shared by all tissues but display a tissue-specific activity that is mediated by in trans factors. It is tempting to speculate that the same neo-ARE that is shared by all cells in our patients similarly exerts a tissue specific destabilizing effect via yet unidentified tissue-specific in trans factors. Although ZFP36, which we show mediates at least part of the destabilizing effect created by the neo-ARE, does not appear to be tissue-specific in distribution according to published data, we do not rule out the possibility that it may display variable abundance in different tissues. Alternatively, a cornea-specific non-coding RNA is another possible culprit since tissue specificity of many micro-RNA species is well documented. Finally, it is also possible that previously reported coding mutations in SCL4A11 result in dysfunctional proteins whereas our neo-ARE mutation only affects abundance with resulting tissue-specific threshold-dependent phenotype. This would be consistent with the fact that the 15 previously reported SLC4A4 mutations (11 missense mutations, two stopgain, and two deletion mutations) always manifested clinically in a syndromic fashion comprising renal tubular acidosis and ocular abnormalities as well as varying intellectual and growth abnormalities. Consistent with our hypothesis, none presented with isolated phenotypes.
In conclusion, we report the first point ARE-creating mutation to cause a Mendelian phenotype. The creation of a neo-ARE as a result and the tissue-specific phenotypic expression of an otherwise pleiotropic disease gene suggests a novel mechanism for variable expressivity of human diseases. Investigating the role of ARE in the spatial, in addition to its established role in temporal, control of transiently expressed genes will be an important future direction.
We thank the patients and their families for their enthusiastic participation. We thank the Genotyping and Sequencing Core Facilities at KFSHRC for their technical help. We are also grateful to Shahad Alazahrani for her technical help.
This work was funded in part by KSCDR grant (FSA) and the Saudi Human Genome Program, KACST.
All authors carried out the collection and analysis of data. NP, AOK, KSAK, and FSA wrote the manuscript. All authors read and approved the final manuscript.
Ethics approval and consent to participate
This study was IRB-approved (KFSRHC RAC# 2070023). All subjects have given written informed consent and all experimental methods comply with the Helsinki Declaration.
The authors declare that they have no competing interests.
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