- Open Access
c.3623G > A mutation encodes a CFTR protein with impaired channel function
© Zhang et al. 2016
Received: 16 October 2015
Accepted: 19 January 2016
Published: 22 January 2016
The aims of this study were to characterize clinical features of a pediatric African-American cystic fibrosis (CF) patient heterozygous for F508del and a novel c.3623G > A mutation, and to identify the molecular defect(s) associated with c.3623G > A mutation.
The medical record of this patient was analyzed retrospectively. Western blotting and iodide efflux assay were used to study mutant CFTR protein expression level, maturation status, channel function, and the effects of CFTR modulation on these characteristics.
The encoding protein of c.3623G > A mutation, G1208D-CFTR, has a moderate processing defect and exhibits impaired channel function, which were partially rescued by using VX-809 or exposed to low temperature (28 °C). The patient has mild CF disease manifestations.
Our biochemical findings correlate with the clinical phenotype and suggest that c.3623G > A is a CF-causing mutation. The study helps expand our knowledge of rare CFTR mutations in a minority population and may have important clinical implications for personalized therapeutic intervention.
Cystic fibrosis (CF) is an autosomal recessive genetic disease caused by the loss or dysfunction of the CF transmembrane conductance regulator (CFTR) channel activity resulting from mutations [1, 2]. Clinically, chronic lung disease is the main cause of morbidity and mortality for CF patients. Other symptoms include pancreatic insufficiency, elevated sweat electrolytes, gastrointestinal disorders, reproductive abnormalities, etc. [3, 4].
CFTR is a cAMP/cGMP-regulated chloride /bicarbonate channel primarily expressed at the apical membrane of epithelial cells lining airway, gut, and exocrine glands, where it is responsible for transepithelial fluid secretion and homeostasis [5–7]. CFTR channel function is determined by the number of channels at the cell surface, the open probability of the channels, and the single channel conductance. Mutations in the CFTR gene alter one or more of these parameters, causing the impairment or loss of the channel activity. More than 2000 CFTR mutations have been identified, which can be roughly categorized into 5 groups based on the nature of defect(s) . The classification of CFTR mutations helps define strategies to restore CFTR channel function based on mutation-specific defect(s). It should be noted that some mutations have multiple defects. For example, F508del, the most prevalent CFTR mutation, induces a maturation defect in CFTR protein; when this maturation defect is rescued, the mutant protein still exhibits defects in channel gating and stability at the cell surface. Among the 2000 plus known CFTR mutations, only a relatively few have been studied in detail both at the molecular level and for the specific disease manifestations. In order to better understand the disease of CF and develop effective therapies, there is a need to study the molecular characteristics of rare CFTR mutations to identify the defect(s), particularly for rare mutations seen in minority populations such as African-Americans.
In addition to therapies targeting the downstream disease consequences (symptoms), recent advancements to target the mutant CFTR proteins (CFTR modulation) have potentially revolutionized CF care. Kalydeco™ (also known as ivacaftor or VX-770) was approved by U.S. Food and Drug Administration (FDA) to treat CF patients age 2 or older with G551D and other nine class III and IV mutations . More recently, FDA approved Orkambi™ (a combination of ivacaftor and lumacaftor (also known as VX-809)) to treat CF patients age 12 or older with two copies of F508del .
Here, we present a clinical case of a pediatric African-American CF patient who is heterogeneous for F508del and a novel missense mutation, c.3623G > A. The patient had mild disease manifestations. Search in the available databases [10–12] did not yield any information on this mutation. The goals of this study were to characterize this novel mutation at the molecular level to identify the nature of defect(s), and to explore the possibility of using mutation-specific therapy for potential interventions.
This individual received standard care at The University of Tennessee Cystic Fibrosis Research and Care Center at LeBonheur Children’s Hospital (Memphis, TN, USA). The medical record was analyzed retrospectively after expedited IRB approval (UTHSC 13-02779-XM).
Genotyping was performed at Ambry Genetics (Aliso Viejo, CA, USA) that showed F508del mutation on one chromosome and c.3623G > A on the other.
Diagnostic sweat chloride testing was performed on the patient by using pilocarpine iontophoresis for duplicate samples from right to left arms. Collection was performed using the filter paper method according to CF Foundation/NCCLS guidelines . The chloride concentrations were measured by using a digital chloridometer (Labconco, Kansas City, MO, USA) with a minimal sweat weight of 75 mg.
Antibodies and reagents
Antibodies were purchased from the following companies: Anti-CFTR, clone MM13-4 (EMD Millipore Corporation, CA, USA), anti-β-Actin (Sigma, MO, USA). VX-809 was purchased from Selleckchem (TX, USA). Other reagents used were purchased either from Sigma or Fisher Scientific (PA, USA) at their highest possible purity.
Forward: 5′CTGGCCCTCAGGGGACCAAATGACTGTCAAAG 3′ (GGC > GAC, amino acid G > amino acid D)
Reverse: 5′CTTTGACAGTCATTTGGTCCCCTGAGGGCCAG 3′
All sequences were confirmed at the Molecular Resource Center at The University of Tennessee Health Science Center.
Cell culture and transfection
HEK293 cells were used to express WT and mutant CFTRs. The cells were cultured in DMEM/F12(1:1) (Invitrogen, Grand Island, NY, USA) medium supplemented with 1 % penicillin-streptomycin (Invitrogen) and 10 % Fetal bovine serum (Invitrogen) at 37 °C in 5 % CO2 incubator unless otherwise stated. Lipofectamine 2000 (Invitrogen) was used to transfect the cells following the instruction provided by the manufacturer. At 48 h post-transfection, the cells were used for western blotting or iodide efflux assay.
Cells were lysed in lysis buffer (1× PBS, containing 0.2 % Triton-X-100 and protease inhibitors phenylmethylsulfonyl fluoride (1 mM), pepstatin A (1 μg/ml), leupeptin (1 μg/ml), aprotinin (1 μg/ml)) for 30 min at 4 °C. The lysates were centrifuged at 12,000 rpm for 15 min at 4 °C. The clear supernatants (the total protein levels were measured by using Bradford protein assay) were mixed with 4× sample buffer, denatured, subjected to SDS-PAGE on 5–14 % Gel (Bio-rad, Hercules, CA, USA), and transferred to PVDF membranes. The membranes were blocked with 5 % milk (in 0.1 % PBS-T) and then probed for CFTR (1:1,000 dilution) and β-actin (the loading control, 1:5,000 dilution) using the respective antibodies. The protein bands were detected using ECL™ Western blot detection reagents (GE Healthcare, Buckinghamshire, UK). The densities of bands were quantified using Image J software.
Real-time PCR to measure CFTR mRNA levels
The primers for human GAPDH were:
The PCR thermocycling parameters were: 95 °C for 5 min, and 40 cycles of 95 °C for 10 s, and 60 °C for 30 s. All samples were run in triplicate and levels of CTFR messages were normalized to GAPDH.
Iodide efflux essay
The assay was performed as previously reported . Briefly, cells were grown on poly-lysine-coated 60-cm culture dishes and transiently transfected with WT-, G1208D-, or empty vector using Lipofectamine 2000. After 48 h, the cells were loaded for 60 min at room temperature with the loading buffer (136 mM NaI, 137 mM NaCl, 4.5 mM KH2PO4, 1 mM CaCl2, 1 mM MgCl2, 10 mM glucose, 5 mM HEPES, pH 7.2). Extracellular NaI was washed away thoroughly (5 times) with the efflux buffer (136 mM NaNO3 replacing 136 mM NaI in the loading buffer) and cells were equilibrated for 1 min in a final 1-ml aliquot of the efflux buffer. The first four aliquots were used to establish a stable baseline in efflux buffer alone. PKA activating agonists cocktail (10 μM forskolin, 200 μM CPT-cAMP, and 100 μM IBMX) was added to the efflux buffer and samples were collected every minute for 6 times in the continued presence of agonists. The iodide concentration of each sample was determined using an iodide-sensitive electrode (Orion Research Inc., Beverly, MA, USA) and the efflux rates were reported as nano-moles (nmol)/min. After experiments, the cells were lysed and the total protein concentrations measured. The maximal iodide efflux rates of samples were normalized to their total protein concentrations of cell lysates.
The data were presented as Mean ± S.E.M. Statistical analyses were performed using Student’s t-test and P values < 0.05 were considered significant.
Clinical case summary
The patient was identified after positive newborn screening by the state of Tennessee. The African-American infant was a product of a twin gestation born preterm at 31 weeks. The newborn screening result of this child was positive, with initial elevated immunoreactive trypsinogen of 148 ng/ml and repeat at 3 weeks of age again elevated at 123 ng/ml. At 2 months old, the sweat chloride levels were 51, 45 mmol/L and pancreatic elastase level was low at 116 μg/g (pancreatic insufficiency). Based on these lab testing results and poor weight gain, the child was diagnosed with CF and management was started, including enzyme replacement therapy. The child has had poor but steady weight gain. The sweat chloride levels were 47, 46 mmol/L at 5 months of age and 54, 48 mmol/L at 29 months of age. Stool elastase testing was >500 μg/g at 25 months of age, and pancreatic enzymes supplementation was stopped. Chest radiograph showed normal findings. There have been no admissions for pulmonary exacerbations, and throat cultures have shown growth of only gram-positive organisms. At 35 months old, the child’s height and weight were at the 5th and below the 3rd percentile, respectively. DNA sequencing test revealed that the child is heterozygous for F508del and a missense mutation, c.3623G > A.
c.3623G > A encoding protein, G1208D-CFTR, has defect in maturation and shows impairment in channel function
We next tested the channel function of G1208D-CFTR in HEK293 cells using iodide efflux assay. HEK293 cells transfected with WT-CFTR or vector were used as controls. As shown in Fig. 1d, upon stimulation, WT-CFTR exhibited a typical CFTR-mediated iodide efflux profile  whereas the vector-expressing cells did not show measureable iodide efflux. Although G1208D-CFTR showed a response, the magnitude was markedly smaller compared to WT-CFTR. The maximal iodide efflux rate of G1208D-CFTR was found to be 33 % of that of WT-CFTR (Fig. 1e). The data demonstrates that the channel function of G1208D-CFTR is impaired, which correlates with our finding that the CFTR protein has defect in maturation.
G1208D-CFTR can be partially rescued by exposure to low temperature or using VX-809
We then tested whether VX-809 potentiates the G1208D-CFTR channel function in HEK293 cells using iodide efflux assay. We found that VX-809 did augment the channel function of G1208D-CFTR, with a 1.5-fold increase in the maximal iodide efflux rate compared to DMSO control (Fig. 2f, g).
Newborn screening programs have facilitated the identification of rare or unique CFTR mutations in populations such as Africa-Americans where classical CF presentations are uncommon [16, 17]. Many of these rare mutations have not been well characterized with regard to CFTR channel function and there is a risk that mutations that potentially respond to CFTR-modifying therapies may not be identified in these populations.
Our biochemical findings demonstrate that G1208D-CFTR has a moderate processing defect, characterized by features of impaired CFTR protein maturation and channel function, as well as sensitivity to temperature and responsiveness to correction with VX-809. Although it is well known that variables in genetic background (e.g. modifier genes) and environment factors also affect CF disease manifestations , our finding that G1208D-CFTR has residual CFTR function (33 % of normal CFTR) correlates well with the mild disease phenotype in this patient, with preserved pancreatic function and intermediate sweat chloride levels, when paired with a classical CFTR mutation like F508del.
Our patient is still too young to evaluate the effect of the mutation on lung damage but it has been known that patients with residual CFTR channel function can still develop bronchiectasis with chronic sino-pulmonary infections and other CF-related diseases (e.g., recurrent pancreatitis, CF-related diabetes, male infertility) when they age . Given that the two mutations this patient has, F508del and c.3623G > A, are both responsive to VX-809, we speculate that VX-809 and similar CFTR modulators could be beneficial for his therapy.
We report the clinical features of a pediatric CF patient heterozygous for F508del and a novel missense c.3623G > A mutation. We characterized c.3623G > A mutation at the molecular level using cell culture models and found that the mutant protein has a moderate processing defect and an impaired channel function, which correlates with the mild disease phenotype present in this patient. Our study suggests that c.3623G > A mutation is a mild CF-causing mutation. We also found that the mutant protein can be partially rescued by using a CFTR corrector VX-809 or exposed at a low temperature. Our findings expand our knowledge of rare CFTR mutations, demonstrate that VX-809 restores function to other rare mutations in addition to F508del, and may have clinical implications for possible therapeutic interventions for this and other patients with c.3623G > A mutation.
We thank Dr. Douglas M. Cyr (University of North Carolina, Chapel Hill, NC, USA) for his kindly providing pcDNA3.1-WT-CFTR and pcDNA3.1-F508del- CFTR plasmids. We are grateful to Dr. Anjaparavanda P Naren (Cincinnati Children’s Hospital Medical Center, Cincinnati, OH, USA) for his suggestions and comments on this project. We also thank Dr. Amanda Preston (Scientific Editor, Children’s Foundation Research Institute, Le Bonheur Children’s Hospital, Memphis, TN, USA) for editing the manuscript. Weiqiang Zhang is supported by a U.S. National Institutes of Health (NIH) grant R01 HL123535.
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