Haematologica
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Published online 25 August 2008
Haematologica, Vol 93, Issue 10, 1505-1513 doi:10.3324/haematol.12934
Copyright © 2008 by Ferrata Storti Foundation
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Disorders of Coagulation

Molecular characterization of three novel splicing mutations causing factor V deficiency and analysis of the F5 gene splicing pattern

Claudia Dall'Osso1, Ilaria Guella1, Stefano Duga1, Nadia Locatelli1, Elvezia Maria Paraboschi1, Marta Spreafico2, Abdolreza Afrasiabi3, Christoph Pechlaner4, Flora Peyvandi2, Maria Luisa Tenchini1, Rosanna Asselta1

1 Department of Biology and Genetics for Medical Sciences, University of Milan, Italy
2 A. Bianchi Bonomi, Hemophilia and Thrombosis Center, University of Milan and Department of Medicine and Medical Specialties, IRCCS Maggiore Hospital, Mangiagalli and Regina Elena Foundation, Milan, Italy
3 Hemostasis and Thrombosis Unit, Haematology Research Center, Shiraz Medical University of Science, Shiraz, Iran
4 Innsbruck Medical University, University Hospital, Department of Internal Medicine, Innsbruck, Austria

Correspondence: Rosanna Asselta, Ph.D., Department of Biology and Genetics for Medical Sciences, University of Milan, via Viotti 3/5, 20133 Milan, Italy. E-mail:rosanna.asselta{at}unimi.it


   ABSTRACT
TOP
 ABSTRACT
Introduction
 Design and Methods
 Results
 Discussion
 References
 
Background: Factor V deficiency is a rare autosomal recessive hemorrhagic disorder, associated with bleeding manifestations of variable severity. In the present study, we investigated the molecular basis of factor V deficiency in three patients, and performed a comprehensive analysis of the factor V gene (F5) splicing pattern.

Design and Methods: Mutational screening was performed by DNA sequencing. Wild-type and mutant F5 mRNA were expressed by transient transfection in COS-1 cells, followed by reverse-transcriptase polymerase chain reaction and sequencing. Real-time reverse-transcriptase polymerase chain reaction was used to evaluate degradation of mRNA carrying premature termination codons.

Results: Mutational screening identified three hitherto unknown splicing mutations (IVS8+6T>C, IVS21+1G>A, and IVS24+1_+4delGTAG). Production of mutant transcripts in COS-1 cells demonstrated that both IVS21+1G>A and IVS24+1_+4delGTAG cause the activation of cryptic donor splice sites, whereas IVS8+6T>C causes exon-8 skipping (F5-{Delta}8-mRNA). Interestingly, F5-{Delta}8-mRNA was also detected in wild-type transfected samples, human liver, platelets, and HepG2 cells, demonstrating that F5 exon-8 skipping takes place physiologically. Since F5-{Delta}8-mRNA bears a premature termination codons, we investigated whether this transcript is subjected to nonsense-mediated mRNA decay degradation. The results confirmed the involvement of nonsense-mediated mRNA decay in the degradation of F5 PTC+ mRNA. Moreover, a comprehensive analysis of the F5 splicing pattern led to the identification of two in-frame splicing variants resulting from skipping of exons 3 and 5–6.

Conclusions: The functional consequences of three splicing mutations leading to FV deficiency were elucidated. Furthermore, we report the identification of three alternatively spliced F5 transcripts.

Key words: factor V deficiency, F5, splicing mutations, nonsense-mediated mRNA decay, exon skipping, premature termination codons.


   Introduction
TOP
 ABSTRACT
 Introduction
Design and Methods
 Results
 Discussion
 References
 
Factor V (FV) deficiency (Mendelian Inheritance in Man +227400) is a rare inherited coagulation disorder, characterized by low or unmeasurable levels of FV antigen and coagulant activity.1 This bleeding disorder has a prevalence of about one per million in the general population.2 The clinical manifestations range from mild to severe3 and include epistaxis, menorrhagia, easy bruising, and hemorrhages after trauma, surgery or dental extractions. Hemarthroses and hematomas occur in only one-quarter of the patients, and life-threatening bleeding episodes in the gastrointestinal tract and in the central nervous system are rare. Since no commercial FV concentrate is available, the treatment of this coagulation deficiency relies on the infusion of fresh-frozen plasma.2

The gene coding for human FV (F5) comprises 25 exons, covers a genomic region of 74.5 Kb and maps to chromosome 1q24.2 [UCSC Genome Browser, http://genome.ucsc.edu/].4 Its 7-Kb open reading frame codes for a mature protein of 2196 amino acids.5 To date, 42 genetic defects, all located in F5, have been reported as the cause of severe FV deficiency.1,6–11 Among these, only four variations affecting splicing have so far been identified.10,12–14

It has been estimated that one–third of hereditary genetic diseases as well as many forms of cancer are caused by mutations resulting in the generation of transcripts bearing a premature termination codon (PTC+ transcripts) in their open reading frame.15 The evolutionarily-conserved post-transcriptional mechanism by which PTC+ transcripts are selectively detected and degraded has been called nonsense-mediated mRNA decay (NMD).16–18 This pathway acts as a quality control mechanism preventing the expression of potentially deleterious truncated proteins. Despite the fact that NMD was originally discovered in β-thalassemic patients and was subsequently demonstrated to be an important phenotype modulator of many human genetic diseases, including rare inherited coagulation disorders,15,19–22 it is unlikely that it evolved only to protect cells against the production of truncated proteins generated by low frequency random mutations. More probably, NMD has been maintained during evolution with the primary role of degrading aberrant PTC+ mRNA generated as a consequence of routine errors in gene expression such as inefficient or faulty splicing and errors introduced by RNA polymerase II.23 Furthermore, it has been suggested that NMD may play a pivotal role in regulating gene expression: expression profiles of NMD-deficient yeast strains demonstrated that about 10% of the transcriptome had both qualitatively and quantitatively altered expression.24,25 Likewise, comparison of expression profiles of human cells with normal or reduced NMD activity revealed that NMD targets hundreds of genes.26 In this frame, it was suggested that coupling of unproductive alternative splicing and NMD might be a way to regulate gene expression post-transcriptionally,27 even if it is not clear to what extent this mechanism is common within the cell.28

In this paper, we report the identification of three novel splicing mutations causing FV deficiency. In vitro expression experiments were used to perform studies at the mRNA level, and the contribution of NMD in regulating the amount of a naturally skipped F5 mRNA was investigated in HepgG2 cells. In addition, we provide the first overview of alternative splicing events of the entire F5 mRNA.


   Design and Methods
TOP
 ABSTRACT
 Introduction
 Design and Methods
Results
 Discussion
 References
 
This study was approved by the Institutional Review Board of the University of Milan and was conducted according to the Declaration of Helsinki. Samples were obtained from the analyzed individuals after acquiring appropriate informed consent.

Materials
Oligonucleotides were purchased from Sigma (St. Louis, MO, USA). Their sequences, when not reported, are available on request.

The pMT2/FV mammalian expression plasmid, containing the full-length FV complementary DNA (cDNA), was kindly provided by Dr R.J. Kaufman (Howard Hughes Medical Institute, University of Michigan Medical School, Ann Arbor, USA). Puromycin, cycloheximide, and wortmannin were purchased from Sigma and resuspendend to a concentration of 1 mg/mL in water, 10 mM in dimethyl sulfoxide (DMSO), and 100 mg/mL in DMSO, respectively.

Coagulation tests
FV activity and antigen plasma levels were measured as described elsewhere.20 Briefly, the functional assay was based on the prothrombin time; FV antigen levels were determined using a sandwich enzyme immunoassay, based on a sheep anti-human polyclonal antibody (Affinity Biologicals, Hamilton, ON, Canada). In both assays, the FV level was expressed as a percentage of the level in control plasma pooled from 40 normal individuals, set as 100%. Normal ranges for FV coagulant activity (FV:C) and antigen (FV:Ag) levels were 58–140% and 64–139%, respectively. In plasma, the sensitivity of the functional and immunological tests was 1% and 0.01%, respectively.

DNA extraction, polymerase chain reaction amplifications, and sequencing
Genomic DNA was extracted from blood samples using the Nucleon BACC1 Kit (Amersham Pharmacia Biotech, Uppsala, Sweden) and PCR-amplified under standard conditions, using sense and antisense primers designed on the basis of the known sequence of the F5 gene (GenBank, accession number Z99572) and REDTaq DNA polymerase (Sigma). Direct sequencing of purified PCR products was performed on both strands by the fluorescent dideoxy-terminator method (BigDye Terminator Cycle Sequencing Kit, version 3.1; Applied Biosystems, Foster City, CA, USA) and analyzed using an automated multicapillary 3130 DNA sequencer (Applied Biosystems). The Variant Reporter package was used for mutation detection (Applied Biosystems). Primers for sequencing were the same as in the amplification reactions, except those used for the 2820-bp-long exon 13, which was sequenced using additional internal primers.

Computer-assisted splice-site prediction
Computer-assisted analysis for splice-site prediction was accomplished using the Neural Network Promoter Prediction Tool (NNPPT) program (http://www.fruitfly.org/seq_tools/splice.html) and the NetGene2 (release 2.4) program (http://www.cbs.dtu.dk/services/NetGene2).

Minigene construction and mutagenesis
Three F5 regions were PCR-amplified from the genomic DNA of a healthy individual using the Expand 20 KbPLUS PCR System (Roche Applied Science, Indianapolis, IN, USA) according to the manufacturer’s instructions. Primer couples (F5-In6-F and F5-In9-R, F5-In19-F and F5-In22-R, and F5-In22-F and F5-3’UTR-R) used for these long-range amplifications are reported in Table 1. PCR products were inserted into the pTARGET vector using the pTARGET Mammalian Expression T-Vector System Kit (Promega, Milan, Italy). Plasmids were isolated using the QIAprep Spin Maxiprep Kit (Qiagen, Hilden, Germany), and the recombinant constructs, hereafter referred to as pT-F5(In6-In9)-wt, pT-F5(In20-In22)-wt, and pT-F5(In22-3’UTR)-wt, were checked by sequencing. The three identified mutations were introduced into the relevant wild-type construct by means of the QuickChange Site-Direct Mutagenesis Kit (Stratagene, La Jolla, CA, USA), as instructed by the manufacturer. The three mutant plasmids (namely pT-F5(In6-In9)-IVS8+6T>C, pT-F5(In20-In22)-IVS21+1 G>A, and pT-F5(In22-3’UTR)-IVS24+1_+4delGTAG) were checked by sequencing and extracted as described above.


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  		Table 1. Primers used for RT-PCR and long-range PCR.

 
The pMT2/FV plasmid was used as a template to obtain by mutagenesis a plasmid bearing the deletion (80-bp long) predicted to result from the IVS24+ 1_+4delGTAG mutation. The resulting mutant plasmid (pMT2/FV-{Delta}80bp) was checked by sequencing and extracted as described above.

Cell cultures, transfections, metabolic labeling, and immunoprecipitation
Human hepatoma HepG2 cells, human cervical carcinoma HeLa cells, and African green monkey kidney COS-1 cells were cultured in Dulbecco’s modified Eagle’s medium (DMEM), supplemented with 10% fetal bovine serum. Glutamine (1%) and antibiotics (100 IU/mL penicillin and 100 µg/mL streptomycin) were added to the medium. Cells were grown at 37°C in a humidified atmosphere of 5% CO2 and 95% air and cultured according to standard procedures.

For the in vitro analysis of splicing products, each minigene construct was transiently transfected in HeLa cells by the calcium phosphate technique, essentially as described peeviously.29 Recombinant FV molecules were expressed by transient transfection with the Lipofectamine 2000 reagent (Invitrogen, Carlsbad, CA, USA), as described elsewhere.30 Cell lysates and conditioned media were prepared and immunoprecipitations carried out as described by Duga et al.30 The immunoprecipitated proteins were resolved by 6% sodium dodecyl sulphate-polyacrylamide gel electrophoresis (SDS-PAGE) under non-reducing conditions. Gels were dried under vacuum at 80°C for 1 hour. The labeled proteins were visualized by exposing gels overnight to a storage phosphor screen (Amersham Pharmacia Biotech) and analyzed using a Typhoon 9200 phosphor imager (Amersham Pharmacia Biotech).

Inhibition of the NMD pathway
HepG2 cells were plated at a density of 5.5x106 per 10-cm dish and, after 72 hours, treated with three inhibitors of NMD (puromycin, cycloheximide, and wortmannin): puromycin and cycloheximide block NMD by interfering with protein synthesis, whereas wortmannin selectively inhibits phosphatidylinositol 3-kinase (PI3K), a kinase that is able to phosphorylate PI-3-kinase-related kinase SMG-1 (SMG1) which, in turn, phosphorylates up-frameshift suppressor 1 (Upf1), a regulator of nonsense transcripts which plays a pivotal role in NMD. Puromycin, used at the concentration of 100 µg/mL, was applied to cells for 8 hours, whereas both cycloheximide (100 µg/mL) and wortmannin (20 µM) were applied to cells for 4 hours.

After the treatment, cells were washed twice with PBS and total RNA was extracted as described below. Non-treated samples were incubated with the corresponding drug solvent.

RNA extraction and reverse transcriptase-polymerase chain reaction
Total RNA was isolated from platelets, HeLa, and HepG2 cells using the RNAWIZ reagent (Ambion, Austin, TX, USA). Liver RNA was extracted by the acid guanidinium thiocyanate–phenol–chloroform method described by Chomczynski and Sacchi.31 Random non-amers and the Enhanced Avian RT-PCR Kit (Sigma) were used to perform first-strand cDNA synthesis starting from 1.5 µg of total RNA, according to the manufacturer’s instructions. Of a total 20-µL mixture, 1-2.5 µL were used as a template to amplify wild-type and mutant transcripts, using exonic primer couples (Table 1). PCR were carried out using REDTaq DNA polymerase under standard conditions.

Real-time RT-PCR
Real-time PCR assays were performed using the iQ5 real-time PCR detection system (Biorad, Hercules, CA, USA) and the iQ SYBER Green Supermix kit (Biorad) according to the manufacturer’s instructions. In each reaction, 1.5 µL of cDNA from treated or untreated HepG2 cells were used. Differences in F5-{Delta}8-mRNA abundance were quantified by the {Delta}{Delta}CT method.32 The F5 wild-type transcript was used as the reference. Primer couples, designed to specifically amplify F5 transcripts including or not exon 8, are listed in Table 1.


   Results
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 ABSTRACT
 Introduction
 Design and Methods
 Results
Discussion
 References
 
Case reports and laboratory analysis
Three unrelated patients (A, B, and C) affected by FV deficiency were analyzed (Table 2). Patient A is an Iranian woman, born from a consanguineous marriage. Her FV plasma levels were moderately reduced (FV:C= 5% and FV:Ag= 6%); she suffered only from epistaxis and was successfully treated with fresh-frozen plasma. Her siblings did not report any bleeding problems.


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  		Table 2. Clinical and genetic characteristics of the FV-deficient patients analyzed.

 
Patient B was an Italian man from Sassari (Sardinia). At the time of blood sampling he was 54 years old; he died 2 years later from intracranial bleeding due to severe hypertension. No FV activity could be detected in his plasma (<1%), and his FV antigen level was severely reduced (0.1%).

Patient C is a 31-year old woman from Austria, whose FV:C levels were reduced to 3%. She suffered from repeated bleeding, without preceding trauma; she had had frequent nosebleeds (starting at the age of 13 months and ceasing at the age of 7 years), had repeated muscle hemorrhages in the lower limbs, a gastrointestinal hemorrhage (at the age of 10 years), and macrohematuria. She also presented with spleen rupture, treated with splenectomy. None of her relatives was reported to have bleeding problems.

Mutational screening
The whole coding region, all intron-exon boundaries, and about 300 bp of the promoter region of the F5 gene were PCR-amplified from the patients’ genomic DNA. Direct sequencing of all amplified fragments allowed us to identify five genetic defects, three of which were hitherto unknown (IVS8+6T>C, IVS21+1G>A, and IVS24+1_+4delGTAG) while the other two had been previously described [g.75002G>A, leading to the Arg2074His missense substitution,33 and g.51452C>T, causing the Arg1002ter nonsense mutation]34 (Table 2). IVS8+6T>C was the only mutation found in the homozygous state in patient A, while patients B and C were compound heterozygotes for the IVS21+1G>A and Arg1002ter, and for the IVS24+1_+4delGTAG and Arg2074His mutations, respectively. The two already described genetic defects were not further investigated, whereas the three putative splicing mutations, whose absence in the general population was verified by sequencing 200 haploid genomes, were characterized in depth.

Splice-site predictions
The effect of the predicted splicing mutations (IVS8+6T>C, IVS21+1G>A, and IVS24+1_+4delGTAG) was first analyzed by computer-assisted splice-site prediction using the NNPPT and NetGene 2 programs. As far as the IVS8+6T>C mutation is concerned, both programs recognized the wild-type as well as the mutant splice site without any appreciable score reduction (0.98 vs. 0.99 and 0.94 vs. 0.90 for the NNPPT and NetGene2, respectively). Conversely, no donor splice site was identified, either in the wild-type or in the mutant sequence, in the region surrounding the IVS21+1G>A mutation. Finally, this in silico analysis detected the wild-type donor splice site of exon 24 with a score of 0.68 using the NNPPT and of 0.92 with NetGene2, whereas the mutant sequence was no longer identified as a donor splice site.

Production of F5 mRNA in HeLa cells
To examine the effects of the IVS8+6T>C, IVS21+1G>A, and IVS24+1_+4delGTAG mutations on F5 pre-mRNA splicing, appropriate F5 minigene constructs (namely pT- F5(In6-In9)-wt, pT- F5(In20–In22)-wt and pT- F5(In22-3’UTR)-wt) were generated, by cloning the relevant PCR-amplified genomic fragment into the mammalian expression vector pTARGET (Figure 1A, B, C left panels). The orientation of the inserts and absence of unanticipated changes due to PCR errors in the cloned regions were checked by sequencing. Subsequently, these three vectors were subjected to site-directed mutagenesis to obtain recombinant constructs containing the identified defects.


Figure 1931505
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  		Figure 1. Functional analysis of the effect of IVS8+6T>C, IVS21+1G>A, and IVS24+1_+4 delGTAG mutations on F5 pre-mRNA splicing. (A,B,C) Left panels: Schematic representation of the F5 regions cloned to produce minigene constructs. Exons (numbered) are indicated by boxes, introns are represented by lines and are not to scale. Primers used in cloning experiments are indicated by arrows showing the primer orientation. Middle panels: RT-PCR products obtained from RNA of cells transfected with the relevant minigene construct, separated on a 2% agarose gel (primer couples are listed in Table 1). Lane M: molecular weight marker (pUC98-HaeIII); lanes 1 and 2: RT-PCR products amplified from transfected HeLa cells expressing wild-type and mutant constructs, respectively. Right panels: schematic representation of normal (above) and aberrant (below) splicing events. The three mutations identified are indicated by arrows. In the panels in B and C the cryptic donor splice sites activated by the mutations are shaded in gray and the skipped portions of exons 21 and 24 are indicated by a curly bracket.

 
Wild-type and mutant plasmids were independently transfected in HeLa cells (not expressing FV). Total RNA was extracted after 48 hours and RT-PCR assays were performed to analyze the splicing pattern of both wild-type and mutant transcripts (Figure 1): all mutant minigene constructs gave rise to fragments with different electrophoretic mobility compared to that of the wild-type ones. In particular, the RT-PCR product derived from the IVS8+6T>C mutant vector was approximately 180 bp shorter than the wild-type one, and direct sequencing of this fragment demonstrated that the entire exon 8 was skipped from the mature mRNA (Figure 1A middle and right panels). RT-PCR analyses demonstrated that transcripts produced from the IVS21+1G>A and IVS24+1_+4delGTAG mutant plasmids (approximately 100 and 80 bp shorter than the wild-type ones) were generated by the use of cryptic donor splice sites located in exons 21 and 24, respectively (Figure 1B and C, middle and right panels). In all cases, the splicing defect would result in the introduction of a PTC. It has been demonstrated that PTC located within a distance of 50–55 nucleotides from the last exon-exon junction or located in the last exon fail to trigger this surveillance system.12 Based on this rule, PTC+ mRNA resulting from the IVS8+6T>C and IVS21+1G>A mutations are probably subjected to NMD and consequently will not be translated into a mutant protein, whereas the PTC+ transcript resulting from the IVS24+1_+4delGTAG mutation is supposed not to be detected and degraded by NMD, thus leading to the synthesis of a truncated FV protein (p.Met2120IlefsX12; numbering omits the signal peptide).

Expression of wild-type and mutant recombinant FV in COS-1 cells
The effect of the IVS24+1_+4delGTAG mutation on FV secretion was investigated by in vitro expression of mutant and wild-type FV molecules in COS-1 cells, which do not express endogenous FV. To this purpose, the pMT2/FV expression plasmid, containing the full-length F5 cDNA, was subjected to mutagenesis, to remove the same 80 nucleotides skipped in the IVS24+1_+4delGTAG mutant transcript. Cells were independently transfected with either the wild-type or the mutant plasmid. After labeling with [35S]-methionine and [35S]-cysteine for 16 hours, recombinant FV molecules were collected by immunoprecipitation from culture media and cell lysates. As for the wild-type protein, SDS-PAGE showed normal secretion of the molecule; by contrast, the mutant FV was detectable only intracellularly (data not shown).

Analysis of the F5 splicing pattern
Interestingly, RT-PCR analysis of the effect of the IVS8+6T>C mutation on splicing showed that a PCR fragment with the same electrophoretic mobility as that of the mutant one was also detectable in cells producing the wild-type transcript (Figure 1A middle panel, lane wt). To verify the hypothesis of the existence of alternative physiological splicing, skipping the entire exon 8 (Figure 2A), total RNA extracted from human liver, platelets, and HepG2 cells (normally producing FV) was subjected to RT-PCR analysis. For this analysis, a specific primer couple was designed to amplify only the aberrant mRNA (Table 1). RT-PCR analysis demonstrated that exon-8 skipping took place physiologically in all the samples analyzed (Figure 2C).


Figure 2931505
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  		Figure 2. Analysis of F5 alternative splicing pattern. (A) Schematic representation of the F5 gene exon-intron structure between exons 7 and 9 and of the predicted destiny of normal (above) and aberrant (below) F5 mRNA. Exons (numbered) are indicated by boxes, introns (not to scale) are indicated by lines. The positions of the primer couples used to amplify the wild-type (F5-Ex7/8-F and F5-Ex8-R) as well as the {Delta}8 transcripts (F5-Ex7/9-F and F5-Ex9-R) are indicated. (B) Effect of NMD inhibition on F5 {Delta}8 transcript levels. Real-time RT-PCR assays were used to quantify the increase of {Delta}8 mRNA after treatment of HepG2 cells with the NMD inhibitors cycloheximide (C 4h), wort-mannin (W 4h), and puromycin (P 8h). The F5 wt transcript (i.e. containing exon 8) was used as the reference. In each experiment, untreated samples were used as calibrators. The fold-increases of skipped F5 mRNA due to the treatments are graphically represented by arrows. (C) Top: Schematic representation of the F5 mRNA showing the position of the 24 exon-exon junctions. The overlapping fragments amplified to analyze the F5 splicing pattern are indicated by lines, continuous lines representing amplicons that highlighted the presence of an alternative splicing event. The numbers above the lines indicate the spanned exons. Middle: enlargement of RT-PCR fragments spanning exons 1/5, 4/8, and 7/11. The position of primer couples designed to specifically amplify alternative F5 transcripts, as well as the sizes of expected PCR products are indicated. Bottom: RT-PCR products amplified from total RNA extracted from HepG2 cells, liver, and platelets separated on a 2% agarose gel. Lane M: molecular weight marker (pUC9-HaeIII), lane {Delta}3, {Delta}5–6, and {Delta}8: RT-PCR products resulting from the amplification of alternative F5 mRNA lacking exons 3, 5–6, and 8, respectively. (D) Schematic representation of the three identified alternative F5 transcripts. Exons (boxes) and introns (lines) are drawn to scale. Splicing events are shown by broken continuous and hatched lines (constitutive and alternative splicing, respectively). Skipped exons are in light gray.

 
Since skipping of the entire exon 8 leads to the generation of a PTC, and considering that it was previously demonstrated that F5 is a target of the NMD pathway (at least in pathological conditions, i.e. in FV-deficient patients with truncating mutations),20,21 we decided to investigate whether the physiological exon-8-skipped mRNA (henceforth called F5-{Delta}8-mRNA) is also degraded by this mRNA surveillance system. For this purpose, wortmannin, cycloheximide, and puromycin were used to inhibit NMD in HepG2 cells, in order to upregulate the expression of those transcripts that normally undergo NMD degradation. Total RNA was extracted from treated and untreated HepG2 cells and the relative quantity of F5-{Delta}8-mRNA was assessed by real-time RT-PCR. This analysis demonstrated an increase in the expression of the F5-{Delta}8-mRNA in treated cells. In particular, wortmannin induced a 1.9-, cycloheximide a 1.5- and puromycin a 2.2-fold increase (Figure 2B), confirming that F5-{Delta}8-mRNA is downregulated by NMD.

These results prompted us to analyze the F5 splicing pattern further using total RNA isolated from HepG2 cells treated with puromycin. A set of RT-PCR assays was designed to pick up the vast majority of possible alternative splicing events (Figure 2C). The most interesting results were obtained with RT-PCR assays covering the 5’ region of the F5 mRNA, where three major alternative splice events were detected (data not shown). Their lengths, on the basis of electrophoretic mobility, were compatible with skipping of exons 3, 5–6 , and 8 (as expected). To confirm these predicted skipping events, RT-PCR assays were performed using specific primer couples (Table 1) on human liver, platelet, and HepG2 RNA; the fragments obtained were also subjected to direct sequencing, demonstrating the physiological expression of {Delta}3, {Delta}8, and {Delta}5–6 transcripts in the tissues analyzed (Figure 2C, D). Given that exon 3 and exon 5–6 skipping are in frame, the resulting mRNA do not contain a PTC and are predicted to cause the synthesis of a FV protein lacking 41 (for {Delta}3) and 122 (for {Delta}5–6) amino acids in the A1 domain. As shown in Figure 3, the 41 amino acids encoded by exon 3 form three β-strands involved in the formation of the N-terminal β-sandwich of the domain, whereas the removal of the 122 amino acids caused by exon 5–6 skipping affects almost the whole C-terminal β-sandwich. The 122-residue deletion is also predicted to abolish the disulfide bridge between Cys220 and Cys301, which is involved in stabilizing the entire A1 domain.


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  		Figure 3. Three-dimensional model of human FVa showing the protein regions removed by exon 3 and exon 5–6 in-frame skipping. Ribbon diagram of human FVa, produced using SwissPDB 3.7 software and the coordinates deposited under Protein Data Bank entry 1FV4. The three A domains of FV are shown in blue (A1), red (A2), and yellow (A3), whereas the two C domains are shown in green. The model is oriented to best display the amino acid regions encoded by F5 exon 3 (41 residues) and exons 5–6 (122 residues), which are colored with different shades of light blue. N and C indicate the amino- and carboxy-termini of the heavy and light chains.

 

   Discussion
TOP
 ABSTRACT
 Introduction
 Design and Methods
 Results
 Discussion
References
 
In this work, we studied three unrelated patients with FV deficiency. Laboratory data from blood samples from these three individuals showed reduced FV antigen levels and coagulant activity. The clinical symptoms of all the patients concorded well with the bleeding pattern reported in the literature.3

Among rare inherited bleeding disorders, FV deficiency is one of the least characterized from the molecular point of view, with only 42 genetic defects hitherto described.1,6,11 Most of the genetic abnormalities are nonsense, frameshift or missense mutations, whereas, up to now, only four splicing defects have been fully described.

To unravel the molecular basis of FV deficiency in our patients, we performed a complete mutational screening of the F5 gene, which revealed five point mutations. Two of these mutations (Arg2074His and Arg1002ter) have already been described1,33,34 and were not analyzed further. The remaining three novel defects (IVS8+6T>C, IVS21+1A>G and IVS24+1_+4delGTAG), all located in donor splice sites, were investigated in depth.

Up to 10% of all point mutations causing human genetic diseases result in an mRNA splicing defect [HGMD, Human Gene Mutation Database, http://www.hgmd.cf.ac.uk/ac/index.php].35 In the majority of cases, splicing mutations cause the disruption of a pre-existing splice site, frequently resulting in exon skipping.36 The opposite situation, i.e. the activation of a cryptic splice site by point mutation, is less frequent.37 The F5 splicing mutations so far described are located in intron-8 acceptor [IVS8-2A>G],14 exon-10 donor [1701G>T]12, intron-16 acceptor [IVS16-3G>T],10 and intron-19 donor [IVS19+3A>T]13 splice sites. The IVS16-3G>T mutation was not investigated at the mRNA level (at least as far as can be deduced from reading the English abstract, since the paper is in Chinese) whereas, in the remaining cases, the mutations cause the disruption of the canonical splice sites, leading either to the activation of a cryptic splice site12,14 or to complete exon skipping.13 The only mutation introducing a PTC is the 1701G>T; in fact, both IVS8-2A>G and IVS19+3A>T generate an in-frame transcript coding for a FV mutant protein, with an addition of eight amino acids in the A2 domain and a partial deletion of the C2 domain, respectively.

To predict the possible effect of the newly identified mutations on F5 pre-mRNA splicing, computer-assisted splice-site prediction analysis was performed with two programs available online. These tools recognized a significant difference between the wild-type and the mutant sequence only for IVS24+1_+4delGTAG. Since in silico analyses were partially inconclusive, and considering the impossibility of obtaining biological specimens suitable for RNA extraction from either the patients or their relatives, we decided to study the effects of the identified mutations on F5 splicing using an in vitro approach. This analysis demonstrated that all the splicing mutations inactivate the corresponding donor splice site. In the case of IVS8+6T>C the entire exon 8 is skipped from mature mRNA, whereas IVS21+1G>A and IVS24+1_+4delGTAG both activate a cryptic donor splice site (located in exons 21 and 24, respectively). In all cases, the splicing defect would determine the introduction of a PTC, 1833, 242, and 64 residues before the canonical stop. Considering that it was previously demonstrated that the F5 gene is subjected to NMD,20,21 only mRNA carrying the IVS8+6T>C and IVS21+1G>A mutations are predicted to be degraded by this pathway, their PTC being located before the last exon of F5. In contrast, the IVS24+1_+4delGTAG splicing defect leads to the introduction of a PTC in the last exon of the gene, thus determining the synthesis of a truncated FV protein, whose fate was investigated by in vitro expression experiments. This analysis demonstrated that the FV mutant molecule was not competent for secretion, as expected for FV molecules with partial deletion of the C2 domain.13,38,39 These results clearly demonstrated the causal role of each of the identified mutations in determining FV deficiency.

Interestingly, the molecular characterization of IVS8+6T>C led to the identification of physiological alternative splicing involving skipping of exon 8. The presence of this naturally occurring alternative splicing was confirmed in HepG2 cells, human liver, and platelets. Since exon-8 skipping leads to the generation of a PTC, we decided to investigate whether this F5-{Delta}8-mRNA is indeed degraded by NMD. For this purpose, three inhibitors of NMD were used to treat HepG2 cells and real-time RT-PCR assays were performed to evaluate the possible increase in the aberrant mRNA level in treated vs. untreated samples: in all cases an increase was detected in the expression of the F5-{Delta}8-mRNA. This finding is interesting considering that the action of NMD on F5 transcripts has, up to now, been evaluated only in the case of PTC+ mRNA determined by FV-deficiency-causing mutations20,21 but has never been evaluated on physiologically alternatively spliced transcripts. Furthermore, the identification of the first F5 alternative splicing event associated with NMD suggests that F5 gene expression could be regulated post-transcriptionally by a mechanism coupling alternative splicing and NMD.27,28

To analyze the F5 splicing pattern further, RT-PCR assays covering almost the whole F5 coding sequence were performed. This analysis revealed the occurrence of multiple alternative splicing events; among the various fragments produced, we further characterized the major ones, which, on the basis of their electrophoretic mobility, showed in-frame exon skipping (i.e. exons 3 and 5–6). The presence of these alternative splices was confirmed in human liver and platelets by specific RT-PCR assays followed by direct sequencing of the amplified fragments. Interestingly, for all three naturally occurring alternative splicing events, in silico splice-site prediction analysis of the exons involved in the skipping events revealed that either the acceptor or the donor wild-type splice site was not identifiable, suggesting that the observed aberrant skipping could possibly be related to the weakness of such sites. The predicted FV molecules translated from the F5 {Delta}3 and the {Delta}5–6 transcripts would lack 41 and 122 amino acids, respectively, in the A1 domain. It can be hypothesized that such drastic deletions would perturb packing of the A1 domain, likely affecting protein stability and competence for secretion, as demonstrated for other recombinant FV mutant proteins.13,38,39 Should these proteins be secreted into the circulation, it is conceivable that they would be expressed at extremely low levels, as demonstrated by the very low levels of the transcripts detected in HepG2 cells (data not shown).

In conclusion, we have demonstrated the functional consequences of three novel splicing mutations leading to FV deficiency. Furthermore, the comprehensive analysis of the F5 splicing pattern led to the identification of two in-frame splicing variants and one out-of-frame alternative splicing event, which was demonstrated to be downregulated by the NMD pathway, thus suggesting a possible role of a mechanism coupling alternative splicing and NMD in the regulation of F5 expression.


   Acknowledgments
 
the authors wish to thank Veronica Astro for excellent technical assistance, and Dr. G. Piseddu (Servizio di Coagulazione, Servizio di Prevenzione, Diagnosi e Terapia delle Malattie Emorragiche e Trombotica, Azienda USL n. 1, Sassari, Italy) for clinical identification of the probands, taking the family histories and collecting blood samples. We also thank all members of the families analyzed in this study for their participation.


   Footnotes
 
Authorship and Disclosures

All the authors participated in the conception and design of the present study, in the analysis and interpretation of the data, and in revising the manuscript. CDO, IG, NL, EMP, and MS were responsible for PCR amplifications, sequence analysis, site-directed mutagenesis, expression experiments, and drafting the manuscript. SD participated in the conception of the study, interpretation of the results, and in reviewing the manuscript. MLT was involved in the study design and in the discussion of the results. AA, CP, and FP were responsible for the recruitment and clinical management of the patients. RA participated in writing the manuscript and supervised the entire study. The authors reported no potential conflicts of interest.

Funding: RA is the recipient of a Bayer Hemophilia Early Career Investigator Award 2005. The financial support of PRIN (Programmi di Ricerca Scientifica di Rilevante Interesse Nazionale, Grant n. 2005058307_002) and FIRST (Fondo per gli Investimenti Ricerca Scientifica e Tecnologica) is gratefully acknowledged.

Received for publication February 18, 2008. Revision received June 6, 2008. Accepted for publication June 11, 2008.


   References
TOP
 ABSTRACT
 Introduction
 Design and Methods
 Results
 Discussion
 References
 

  1. Asselta R, Tenchini ML, Duga S. Inherited defects of coagulation factor V: the hemorrhagic side. J Thromb Haemost 2006;4:26-34.[Medline]
  2. Mannucci PM, Duga S, Peyvandi F. Recessively inherited coagulation disorders. Blood 2004;104:1243-52.[Abstract/Free Full Text]
  3. Lak M, Sharifian R, Peyvandi F, Mannucci PM. Symptoms of inherited factor V deficiency in 35 Iranian patients. Br J Haematol 1998;103:1067-9.[CrossRef][ISI][Medline]
  4. Kent WJ, Sugnet CW, Furey TS, Roskin KM, Pringle TH, Zahler AM, et al. The Human Genome Browser at UCSC. Genome Res 2002;12:996-1006.[Abstract/Free Full Text]
  5. Cripe LD, Moore KD, Kane WH. Structure of the gene for human coagulation factor V. Biochemistry 1992;31:3777-85.[CrossRef][ISI][Medline]
  6. Kling SJ, Griffee M, Flanders MM, Rodgers GM. Factor V deficiency caused by a novel missense mutation, Ile417Thr, in the A2 domain. J Thromb Haemost 2006;4:481-3.[CrossRef][ISI][Medline]
  7. Yamakage N, Ikejiri M, Okumura K, Takagi A, Murate T, Matushita T, et al. A case of coagulation factor V deficiency caused by compound heterozygous mutations in the factor V gene. Haemophilia 2006;12:172-8.[CrossRef][ISI][Medline]
  8. Asselta R, Dall’Osso C, Duga S, Spreafico M, Saxena R, Tenchini ML. Coagulation factor V gene analysis in five Indian patients: identification of three novel small deletions. Haematologica 2006;91:1724-6.[Abstract/Free Full Text]
  9. Jones CD, Yeung C, Negro F, Zehnder JL. Molecular characterization and subcellular localization of Tyr478del: a pathogenic in-frame deletion in coagulation factor V. J Thromb Haemost 2007;5:431-3.[CrossRef][ISI][Medline]
  10. Zheng WD, Liu YH, Liu HF, Chen ZH, Wang Y. Identification of two novel mutations of human blood coagulation factor V gene in a Chinese family with congenital factor V deficiency. Zhonghua Yi Xue Yi Chuan Xue Za Zhi 2006;5:515-8.
  11. Caudill JS, Sood R, Zehnder JL, Pruthi RK, Steensma DP. Severe coagulation factor V deficiency associated with an interstitial deletion of chromosome 1q. J Thromb Haemost 2007;5:626-8.[CrossRef][ISI][Medline]
  12. Schrijver I, Koerper MA, Jones CD, Zehnder JL. Homozygous factor V splice site mutation associated with severe factor V deficiency. Blood 2002;99:3063-5.[Abstract/Free Full Text]
  13. Asselta R, Montefusco MC, Duga S, Malcovati M, Peyvandi F, Mannucci PM, et al. Severe factor V deficiency: exon skipping in the factor V gene causing a partial deletion of the C1 domain. J Thromb Haemost 2003;1:1237-44.[CrossRef][ISI][Medline]
  14. Fu QH, Zhou RF, Liu LG, Wang WB, Wu WM, Ding QL, et al. Identification of three F5 gene mutations associated with inherited coagulation factor V deficiency in two Chinese pedigrees. Haemophilia 2004;10:264-70.[CrossRef][Medline]
  15. Frischmeyer PA, Dietz HC. Nonsense-mediated mRNA decay in health and disease. Hum Mol Genet 1999;10:1893-900.
  16. Losson R, Lacroute F. Interference of nonsense mutations with eukaryotic messenger RNA stability. Proc Natl Acad Sci USA 1979;76:5134-7.[Abstract/Free Full Text]
  17. Maquat LE. Nonsense-mediated mRNA decay: splicing, translation and mRNP dynamics. Nat Rev Mol Cell Biol 2004;5:89-99.[CrossRef][ISI][Medline]
  18. Lejeune F, Maquat LE. Mechanistic links between nonsense-mediated mRNA decay and pre-mRNA splicing in mammalian cells. Curr Opin Cell Biol 2005;17:309-15.[CrossRef][ISI][Medline]
  19. Holbrook JA, Neu-Yilik G, Hentze MW, Kulozik AE. Nonsense-mediated decay approaches the clinic. Nat Genet 2004;36:801-8.[CrossRef][ISI][Medline]
  20. Montefusco MC, Duga S, Asselta R, Santagostino E, Mancuso G, Malcovati M, et al. A novel two base pair deletion in the factor V gene associated with severe factor V deficiency. Br J Haematol 2000;111:1240-6.[CrossRef][ISI][Medline]
  21. van Wijk R, Montefusco MC, Duga S, Asselta R, van Solinge W, Malcovati M, et al. Coexistence of a novel homozygous nonsense mutation in exon 13 of the factor V gene with the homozygous Leiden mutation in two unrelated patients with severe factor V deficiency. Br J Haematol 2001;114:871-4.[CrossRef][ISI][Medline]
  22. Soldà G, Asselta R, Ghiotto R, Tenchini ML, Castaman G, Duga S. A type II mutation (Glu117stop), induction of allele-specific mRNA degradation and factor XI deficiency. Haematologica 2005;90:1716-8.[Abstract/Free Full Text]
  23. Maquat LE. Nonsense-mediated mRNA decay in mammals. J Cell Sci 2005;118:1773-6.[Free Full Text]
  24. He F, Li X, Spatrick P, Casillo R, Dong S, Jacobson A. Genome-wide analysis of mRNAs regulated by the nonsense-mediated and 5' to 3' mRNA decay pathways in yeast. Mol Cell 2003;12:1439-52.[CrossRef][ISI][Medline]
  25. Lelivelt MJ, Culbertson MR. Yeast Upf proteins required for RNA surveillance affect global expression of the yeast transcriptome. Mol Cell Biol 1999;19:6710-9.[Abstract/Free Full Text]
  26. Mendell JT, Sharifi NA, Meyers JL, Martinez-Murillo F, Dietz HC. Nonsense surveillance regulates expression of diverse classes of mammalian transcripts and mutes genomic noise. Nat Genet 2004;36:1073-8.[CrossRef][ISI][Medline]
  27. Green RE, Lewis BP, Hillman RT, Blanchette M, Lareau LF, Garnett AT, et al. Widespread predicted nonsense-mediated mRNA decay of alternatively-spliced transcripts of human normal and disease genes. Bioinformatics 2003;19:118-21.[CrossRef]
  28. Pan Q, Saltzman AL, Kim YK, Misquitta C, Shai O, Maquat LE, et al. Quantitative microarray profiling provides evidence against widespread coupling of alternative splicing with nonsense-mediated mRNA decay to control gene expression. Genes Dev 2006;20:153-8.[Abstract/Free Full Text]
  29. Asselta R, Duga S, Simonic T, Mal-covati M, Santagostino E, Giangrande PL, et al. Afibrinogenemia: first identification of a splicing mutation in the fibrinogen {gamma} chain gene leading to a major {gamma} chain truncation. Blood 2000;96:2496-500.[Abstract/Free Full Text]
  30. Duga S, Montefusco MC, Asselta R, Malcovati M, Peyvandi F, Santa-gostino E, et al. Arg2074Cys missense mutation in the C2 domain of factor V causing moderately severe factor V deficiency: molecular characterization by expression of the recombinant protein. Blood 2003;101:173-7.[Abstract/Free Full Text]
  31. Chomczynski P, Sacchi N. Single-step method of RNA isolation by acid guanidiniumthiocyanate phenolchlo-roform extraction. Anal Biochem 1987;162:156-9.[ISI][Medline]
  32. Livak KJ, Schmittgen TD. Analysis of relative gene expression data using real-time quantitative PCR and the 2-{Delta}Ct method. Methods 2001;25:402-8.[CrossRef][ISI][Medline]
  33. Schrijver I, Houissa-Kastally R, Jones CD, Garcia KC, Zehnder JL. Novel factor V C2-domain mutation (R2074H) in two families with factor V deficiency and bleeding. Thromb Haemost 2002;87:294-9.[ISI][Medline]
  34. Montefusco MC, Duga S, Asselta R, Malcovati M, Peyvandi F, Santa-gostino E, et al. Clinical and molecular characterization of 6 patients affected by severe deficiency of coagulation factor V: broadening of the mutational spectrum of factor V gene and in vitro analysis of the newly identified missense mutations. Blood 2003;102:3210-6.[Abstract/Free Full Text]
  35. Krawczak M, Cooper DN. The human gene mutation database. Trends Genet 1997;13:121-2.[CrossRef][ISI][Medline]
  36. Krawczak M, Reiss J, Cooper DN. The mutational spectrum of single base-pair substitutions in mRNA splice junctions of human genes: causes and consequences. Hum Genet 1992;90:41-54.[ISI][Medline]
  37. Talerico M, Berget SM. Effect of 5' splice site mutations on splicing of the preceding intron. Mol Cell Biol 1990;12:6299-305.
  38. Ortel TL, Devore-Carter D, Quinn-Allen M, Kane WH. Deletion analysis of recombinant human factor V. Evidence for a phosphatidylserine binding site in the second C-type domain. J Biol Chem 1992;267:4189-98.[Abstract/Free Full Text]
  39. Zhang JX, Braakman I, Matlack KE, Helenius A. Quality control in the secretory pathway. the role of calreti-culin, calnexin and BiP in the retention of glycoproteins with C-terminal truncations. Mol Biol Cell 1997;8:1943-54.[Abstract/Free Full Text]
  40. Shapiro MB, Senapathy P. RNA splice junctions of different classes of eukaryotes: sequence statistic and functional implications in gene expression. Nucleic Acids Res 1987;15:7155-74.[Abstract/Free Full Text]




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