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Genetic Variation in Genes Associated with Arsenic Metabolism: Lizhi Yu,1 Kelly Kalla,1 Erin Guthrie,1
Amy Vidrine,1 and Walter T. Klimecki1,2 1Arizona Respiratory Center, Tucson, Arizona, USA; 2Southwest
Environmental Sciences Center, Tucson, Arizona, USA Abstract Individual variability in human arsenic metabolism has been reported frequently in the literature. This variability could be an underlying determinant of individual susceptibility to arsenic-induced disease in humans. Recent analysis revealing familial aggregation of arsenic metabolic profiles suggests that genetic factors could underlie interindividual variation in arsenic metabolism. We screened two genes responsible for arsenic metabolism, human purine nucleoside phosphorylase (hNP) , which functions as an arsenate reductase converting arsenate to arsenite, and human glutathione S-transferase omega 1-1 (hGSTO1-1) , which functions as a monomethylarsonic acid (MMA) reductase, converting MMA(V) to MMA(III) , to develop a comprehensive catalog of commonly occurring genetic polymorphisms in these genes. This catalog was generated by DNA sequencing of 22 individuals of European ancestry (EA) and 24 individuals of indigenous American (IA) ancestry. In hNP, 48 polymorphic sites were observed, including 6 that occurred in exons, of which 1 was nonsynonymous (G51S) . One intronic polymorphism occurred in a known enhancer region. In hGSTO1-1, 33 polymorphisms were observed. Six polymorphisms occurred in exons, of which 4 were nonsynonymous. In contrast to hNP, in which the IA group was more polymorphic than the EA group, in hGSTO1-1 the EA group was more polymorphic than the IA group, which had only 1 polymorphism with a frequency > 10%. Populations representing genetic admixture between the EA and IA groups, such as Mexican Hispanics, could vary in the extent of polymorphism in these genes based upon the extent of admixture. These data provide a framework in which to conduct genetic association studies of these two genes in relevant populations, thereby allowing hNP and hGSTO1-1 to be evaluated as potential susceptibility genes in human arsenicism. Key words: arsenic, biotransformation, European ancestry, indigenous American ancestry, hGSTO1-1, hNP, polymorphisms, SNP. Environ Health Perspect 111:1421-1427 (2003) . doi:10.1289/txg.6420 available via http://dx.doi.org/ doi:doi:10.1289/txg.6420 available via http://dx.doi.org/ [Online 21 July 2003] |
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Address correspondence to W.T. Klimecki, Arizona Health
Sciences Center, BRL-Room C112, 1609 N. Warren Ave., Tucson, AZ 85724
USA. Telephone: (520) 626-7470. Fax: (520) 626-5956. E-mail: walt@resp-sci.arizona.edu
*The online version of this article (available at http://www.ehponline.org)
contains Supplemental Material.
This work was supported by National Institute for Environmental
Health Sciences grant ES06694. WTK was also supported by National Heart,
Lung, and Blood Institute grants HL66801, HL66806, and HL67672.
The authors declare they have no conflict of interest.
Received 21 April 2003; accepted 14 July 2003. Arsenic-induced human carcinogenesis remains one of the most perplexing mechanistic
puzzles in contemporary toxicology. Although current animal models of arsenic-induced
carcinogenesis are of equivocal biological relevance, convincing human epidemiologic
data have identified the skin, lung, and bladder as targets of carcinogenesis
caused by chronic exposure to arsenic (Bates et al. 1992). Several potential
carcinogenic mechanisms have been proposed, including inhibition of DNA repair
enzymes, tumor promoter-like induction of proliferation, alteration of DNA methylation,
and clastogenesis (Kitchin 2001). Notwithstanding their lack of in vivo
potency in carcinogenesis assays, arsenic compounds are potent toxicants both
in vitro and in vivo. Biological effects of in vitro or
in vivo exposure to arsenic include apoptosis, protein ubiquitination,
cellular proliferation, oxidative stress, and enzyme inactivation (Asmuss et
al. 2000; Chen et al. 2001; Hunter 2000; Kirkpatrick et al. 2003). Thus, arsenicals
are clearly biologically active, but no definitive relationship has been established
that links carcinogenesis to specific toxic endpoints.
Toxicologists have been able to assemble the key steps of the arsenic biotransformation
pathway by identifying the chemical species of biotransformed arsenic. This
pathway includes several oxidation state changes, successive oxidative methylations,
and at least four metabolites (Vahter 2002). Notwithstanding the lack of specifically
identified carcinogenic mechanisms of action, available evidence suggests that
arsenic biotransformation is likely to be key to arsenic-induced disease. First,
experimental evidence suggests that arsenic metabolism in humans could produce
toxic intermediates and certainly governs the in vivo balance between
chemical arsenic species with high biological potency and those with low biological
potency. Historically, methylation of arsenic has been regarded as a detoxification
mechanism (Abernathy et al. 1999). Within that historical context, detoxification
typically referred to the lower cytotoxic potency of methylated arsenicals,
namely monomethylarsonic acid of valence V [MMA(V)] and dimethylarsinic acid
of valence V [DMA(V)], compared with inorganic arsenic species. In addition
to the differential cytotoxicity between inorganic arsenic and organic arsenic
in the +V valence state, there is differential cytotoxicity between inorganic
arsenic in the +III valence state and inorganic arsenic in the +V valence state.
To complicate matters further, more recently, it has been shown that, as opposed
to the low potency of MMA(V) and DMA(V), MMA(III) and DMA(III) are
potent inducers of apoptosis, cytosolic protein binding, and epithelial hyperplasia
(Thomas et al. 2001). In fact these methylated arsenic (III) compounds may be
the most potent toxicants in the entire metabolic pathway. Although no direct
link exists between arsenic-induced cytotoxicity and arsenic-induced carcinogenesis,
the differential biological activity of arsenic metabolites is probably not
restricted to cytotoxicity. Thus, understanding arsenic metabolism is likely
to be key to a complete understanding of arsenic carcinogenesis.
A second, equally compelling reason to explore arsenic metabolism is the evidence
that the metabolism of arsenic may be genetically influenced, with significant
interindividual variation in arsenic metabolism among humans. Interspecies comparisons
also suggest a genetic component to arsenic metabolism. Comparison of nine different
strains of rats in which liver S9 fractions were exposed to inorganic arsenic
revealed a 2-fold difference between the strain with the lowest rate of arsenic
methylation versus the strain with the highest rate (Thomas et al. 2001). Parallel
experiments corroborated the S9 fraction results with intact hepatocytes from
the nine strains. In experiments examining the rate of formation of methylated
arsenic in hepatocytes taken from different human donors, nearly a 10-fold difference
was observed (Styblo et al. 1999). Although this difference could be due to
conditions surrounding donor organ condition or assay conditions, it is interesting
to note that a comparison of several large studies measuring the distribution
of urinary arsenic metabolites in humans exposed to inorganic arsenic via drinking
water demonstrated a nearly 7-fold difference in the fraction of urinary arsenic
as MMA (Vahter 2000). It is likely that some of this variability is environmental;
however, it is possible that genetic variation may underlie some of the variation
in arsenic metabolism. A role for genetic determinants of arsenic biotransformation
is supported in recent work by Chung et al. (2002), in which familial aggregation
in the pattern of urinary methylated arsenic metabolites was demonstrated in
Chilean families.
A prerequisite in the evaluation of potential genetic determinants of arsenic
metabolism is the development of a comprehensive catalog of genetic variation
in genes whose products are involved in arsenic biotransformation. With such
a catalog, one can test individual or combinations of polymorphic sites for
association with phenotypes related to arsenic biotransformation, such as patterns
of urinary metabolites. This study represents the first systematic polymorphism
screening of two genes involved in arsenic biotransformation, human purine nucleoside
phosphorylase (hNP) and human glutathione S-transferase omega
1-1 (hGSTO1-1). The products of these genes function as arsenate reductase
and MMA, As(V) reductase, respectively (Radabaugh et al. 2002; Zakharyan et
al. 2001). Because a major focus of our laboratory is the local arsenic-affected
population [European ancestry (EA) individuals and Mexican ancestry individuals],
we developed this catalog using two populations of subjects, EA subjects and
indigenous American ancestry (IA) subjects. Because Mexican ancestry individuals
represent predominantly an admixture between Europeans and indigenous Americans,
these two populations make up the primary genetic background of the locally
relevant populations (Cerda-Flores et al. 2002)
Materials and Methods
Subjects
Anonymous
DNA samples from healthy individuals of self-reported ancestry were obtained
from the Coriell Institute (Camden, NJ). Twenty-two samples from individuals
of EA and 24 samples from individuals of IA were studied. EA individuals were
selected from unrelated Centre d'Etude du Polymorphism Humain samples. The geographical
origin of the IA samples consisted of 5 samples from Peru, 9 samples from Mexico,
1 sample from Ecuador, and 9 samples from Brazil. One DNA sample isolated from
chimpanzee was also included in the study. These samples are commercially available;
individual sample identification and ordering information are shown in the Supplemental
Material, Table 1.
Polymerase Chain Reaction
Genomic sequences for hNP and hGSTO1-1 were accessed from the
UCSC Genome Browser (http://www.genome.ucsc.edu)
November 2002 freeze. Polymerase chain reaction (PCR) amplicons were designed
to completely traverse each gene, such that each amplicon was approximately
900 bp long, and consecutive amplicons overlapped each other by approximately
200 bp. PCR reactions contained 20 ng genomic DNA, 1 pmol of each primer, 0.2
U taq polymerase (platinum taq; Invitrogen, Carlsbad, CA) and 0.1 µM deoxynucleotide
triphosphates in a total volume of 10 µL. Specific reaction conditions,
including primer sequences, are available from the authors.
Direct Polymerase Chain Reaction Sequencing
PCR amplicons were prepared for cycle sequencing by diluting them with water,
using a dilution range of 1:3-1:6, depending on the reaction yield determined
by agarose gel electrophoresis. Cycle-sequencing reactions were assembled using
0.4 µL cycle-sequencing premix (BigDye, version 3.0; Applied Biosystems,
Foster, CA), 1 pmol sequencing primer, 1.8 µL 5
sequencing dilution buffer and 5 µL PCR product in a final volume of 10
µL. Cycle-sequencing reactions were purified using DNA-affinity magnetic
beads (Agencourt Biosciences, Beverly, MA). Purified sequencing reactions were
electrophoretically analyzed using a DNA Analyzer 3730 (Applied Biosystems).
Polymorphism Identification and Analysis
Sequence chromatograms were processed for base calling and assembly using
the phred, phrap, and Consed suite of software programs (Ewing et al. 1998;
Gordon et al. 1998). Initial polymorphism tagging was performed using Polyphred,
with a minimum sequence quality of phred 25 (Nickerson et al. 1997). Potential
polymorphic sites initially identified by Polyphred were individually confirmed
by visual inspection of sequence traces. A criterion of this visual inspection-confirmation
was that the polymorphism must be observed in multiple chromatograms from singleton
polymorphisms (polymorphisms occurring in only one subject) or in multiple subjects.
For these confirmed polymorphic sites, each genotype for each subject was also
confirmed by visual inspection of chromatograms. Polymorphic sites and associated
subject-identified genotypes were automatically output to a relational database
for further analysis, which included the automated generation of ethnicity-specific
genotype frequencies, allele frequencies, and goodness-of-fit tests for Hardy-Weinberg
equilibrium. Haplotypes were inferred using a Gibbs-sampling algorithm as implemented
in the Phase software program (Stephens et al. 2001). Because the accuracy of
statistically inferred haplotype increases with increasing haplotype frequency,
we used polymorphisms with a minimum frequency [minor allele frequency (MAF)]
of 0.10 to define relatively common haplotypes (Tishkoff et al. 2000). Pairwise
linkage disequilibrium (LD) was calculated as r2, a measure
of the product-moment correlation coefficient (Devlin and Risch 1995).
Gene Context of Polymorphisms
Each gene was annotated graphically using the Artemis software program (Rutherford
et al. 2000). Annotations included exon location, protein coding exon subset,
reading frame, and polymorphism site. Coding region polymorphisms were evaluated
for codon changes resulting from polymorphisms and the predicted effect on amino
acid sequence.
Results
Glutathione S-Transferase Omega 1-1, MMA(V) Reductase
Based on mapping data from the November 2002 freeze of the Human Genome Browser,
hGSTO1-1 contains six exons and extends for 12,551 bp of chromosome 10,
in banding region q25.1. This is a region of low overall meiotic recombination,
with a sex-averaged rate of 0.6 centimorgan (cM)/megabase (Mb) (Kong et al.
2002). The summary of the results of polymorphism screening in hGSTO1-1
is shown in Figure 1. Overall, 33 polymorphic sites were observed in the approximately
16,000 bases of genomic DNA that we sequenced, including the gene itself, 5´
upstream, and 3´ downstream genomic regions. The flanking sequences of
all polymorphisms are given in Supplemental Material, Table 2,
Figure 1. Summary of frequency
and gene context of polymorphisms discovered in hGSTO1-1 in EA (Europe)
and IA (America) subjects. “ID” column indicates the polymorphism
identification number relative to the location in the consensus sequence,
with the first base of the consensus numbered 1. *Indicates insertion/deletion.
“ATG offset” indicates the polymorphism location relative to
the first base “A” of the ATG methionine initiation codon. “Freq
%” is the MAF, graphically displayed in the column to the right. Nonsynonymous
SNPs are denoted by amino acid substitutions, e.g., A140D. |
Table
2
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Figure 2. Summary of frequency
and functional context of polymorphisms discovered in hNP in EA and IA subjects.
Syn, synonymous SNP. “ID” indicates the polymorphism identification
number relative to the location in the consensus sequence, with the first
base of the consensus numbered 1. *Indicates insertion/deletion. “ATG
offset” indicates the polymorphism location relative to the first
base “A” of the ATG methionine initiation codon. “Freq
%” is the MAF, graphically displayed in the column to the right. Nonsynonymous
SNP are denoted by amino acid substitutions, e.g., G51S. |
Table
3
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Table
4
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to allow unambiguous identification of polymorphisms. Complete genotypes for
every individual at every site are shown in Supplemental Material, Figure 1
(EA population), and Supplemental Material, Figure 2 (IA population). Six polymorphisms
occurred in exons 4 and 6, 2 of which were in the 3´ untranslated region.
The 4 remaining polymorphisms were nonsynonymous, resulting in two nonconservative
amino acid substitutions (A140D, E208K), one amino acid deletion (E155del),
and one conservative amino acid substitution (A236V). An interesting feature
of these data is the distribution of polymorphisms between the EA and IA groups.
Overall, the IA group was minimally polymorphic. The 14 polymorphisms observed
in the IA population had a mean heterozygosity of 0.085 ± 0.064 (mean ±
SD). In contrast, the mean heterozygosity of the 21 polymorphisms observed in
the EA population was 0.223 ± 0.195. In large part the genetic polymorphisms
of each group were exclusive to that group. We observed 19 polymorphisms exclusive
to the EA group, 12 polymorphisms exclusive to the IA group, and only 2 shared
polymorphisms (668 and 8283). LD among high-frequency (MAF > 0.10) polymorphisms
was observed spanning over 11,000 bp in the EA group, with r2
values approaching 1.0 between sites 2609 and 12707. Of the 8 polymorphisms
in the EA group with MAF > 0.10, 7 (890, 1285, 2609, 6398, 8238, 10629, 12707)
were in substantial LD with each other, with r2 values between
0.60 and 1.0. LD in the IA group is difficult to evaluate because of the low
frequency of the polymorphisms. Complete pairwise LD plots for hGSTO1-1
are shown in Supplemental Material, Figure 3 (EA group), and Supplemental Material,
Figure 4 (IA group). The lack of diversity of the IA samples in this genomic
region is also reflected in the haplotype analysis, shown in Tables 1 and 2.
Considering only relatively common haplotypes, here arbitrarily defined as those
composed of polymorphisms with an MAF > 0.10, only two haplotypes defined
the entire IA population. These haplotypes, in turn, were defined by polymorphism
668, the only polymorphism that exceeded this MAF threshold. Thus, 84% of the
chromosomes studied carried the major allele for polymorphism 668. The remaining
16% of the IA chromosomes carried the minor allele for polymorphism 668. Despite
having 8 polymorphisms exceeding the 0.10 MAF threshold, the EA population was
divided into only three primary haplotypes, which represented 93% of all EA
chromosomes (Table 2).The most common EA haplotype, GGG + AACT, was also the
common IA haplotype. The second most common EA haplotype, AAA - GCAC, was
entirely absent from the IA population.
Purine Nucleoside Phosphorylase, Arsenate Reductase
hNP contains six exons and occupies 7,636 bp of chromosome 14 in band
region q11.2. Substantially more meiotic recombination occurs in this region,
compared with hGSTO1-1, with a sex-averaged rate of 3.7 cM/Mb (Kong et
al. 2002). The summary of the results of polymorphism discovery in hNP
is shown in Figure 2. The flanking
sequences of all polymorphisms are given in Supplemental Material, Table 3,
to allow unambiguous identification of polymorphisms. Complete genotypes for
every individual at every site are shown in Supplemental Material, Figure 5
(EA population), and Supplemental Material, Figure 6 (IA population). Forty-eight
polymorphisms were observed in the approximately 11,000 bases of DNA sequenced
in this genomic region. Six polymorphisms occurred in exons, of which 1 (2544)
occurred in the 5´ untranslated RNA (UTR) and 1 (9987) in the 3´ UTR.
Of the remaining 4 polymorphisms, 3 (5483, 5594, 8254) were synonymous, and
1 (5574) resulted in a conservative amino acid substitution (G51S). In contrast
to the situation for hGSTO1-1, in the genomic region of hNP, the
IA group was more polymorphic than was the EA group, with mean heterozygosity
values of 0.292 ± 0.127 for the IA group and 0.200 ± 0.132 for the
EA group. Unlike hGSTO1-1, where 94% of the polymorphisms were exclusive
to one group or the other, only 51% of all hNP polymorphisms were exclusive
to one group, with 11 polymorphisms exclusive to the EA group and 13 polymorphisms
exclusive to the IA group. Twenty-four polymorphisms were shared by both groups.
The contrast in overall variability in the IA group between hGSTO1-1
and hNP was evident in the number of polymorphisms exceeding the 0.10
MAF threshold for haplotype analysis. In contrast to hGSTO1-1 (in which
the IA group had 1 such polymorphism, whereas the EA group had 8), in hNP
the IA group had 30 polymorphisms exceeding this threshold, whereas the EA group
had only 19. LD in both the IA and EA groups was also more complex in hNP;
in each group the high-frequency polymorphisms occurred in no less than three
clusters, with high LD within a cluster but low LD between clusters (data not
shown). Complete pairwise LD plots for hNP are shown in Supplemental
Material, Figure 7 (EA group) and Supplemental Material, Figure 8 (IA group).
The results of haplotype analysis for hNP are shown in Tables 3 and 4.
Haplotype analysis revealed a greater complexity in the IA population within
the hNP genomic region than in hGSTO1-1. Of the 48 IA chromosomes,
91.7% comprised five halotypes. Similarly, the EA population chromosomes could
largely be described by five haplotypes, which accounted for 81.8% of all EA
chromosomes studied.
Discussion
Genetic determinants of interindividual variability in arsenic metabolism
have been speculated upon frequently in the literature, even before specific
arsenic-metabolizing genes were identified (Abernathy et al. 1999; Vahter 1999,
2000). This project focused on a thorough screening of the first two characterized,
arsenic-metabolic genes, with the objective of producing a catalog of commonly
occurring polymorphisms in individuals of EA, IA, and by inference, many individuals
of Mexican ancestry.
The genetics and molecular biology of hNP have been studied extensively
because of the causative role of some nonsynonymous mutations in hNP
in severe combined immunodeficiency syndrome (SCID) (Markert 1991; Sato and
Wakabayashi 1998). Given the severe phenotype of SCID, it is not difficult to
imagine that the spectrum of genetic variations one would observe in the general
population would be confined to a limited range of functional changes in the
protein. In fact for the 92 chromosomes that we studied, we observed only one
nonsynonymous change in the predicted amino acid sequence, a conservative change
of glycine to serine at residue 51. The 5 remaining polymorphisms that occurred
in exons were either synonymous or positioned in untranslated mRNA regions.
Although there is clear selection pressure against amino acid polymorphism in
hNP, it is plausible that genetic polymorphism in gene regulatory regions
could occur, as such changes could manifest themselves in a tissue-specific
manner. Thus, in the presence of a polymorphism occurring in a gene regulatory
region, a lethal target tissue such as T lymphocytes could be spared alterations
in hNP gene expression, while a tissue critical to arsenic metabolism
such as the liver could have altered transcriptional activity. Two polymorphisms,
3207 and 3253, are present within a region of intron 1 that has been defined
as an enhancer element; this element may be absolutely necessary for gene transcription
(Jonsson et al. 1992, 1994). No polymorphisms were observed in the minimal promoter
elements that have been thus far defined for hNP (Jonsson et al. 1991).
hGSTO1-1 is a member of an atypical class of glutathione transferases,
with a biochemical activity more closely resembling glutaredoxins than other,
more typical, glutathione transferase enzymes (Board et al. 2000). Its involvement
in biochemical pathways in the human remains to be fully characterized, but
in addition to its involvement in arsenic biotransformation, hGSTO1-1
may include posttranslational processing of interleukin-1ß (Laliberte
et al. 2003). It is strongly expressed in several tissues, including colon,
heart, liver, ovary, pancreas, prostate, and spleen (Yin et al. 2001).
Our analysis of hGSTO1-1 revealed a higher degree of predicted amino
acid polymorphism than we observed in hNP. As opposed to hNP,
in which only 17% of polymorphisms occurring in exons were nonsynonymous, 67%
(4 of 6) of exon polymorphisms in hGSTO1-1 were nonsynonymous. Of these
4 nonsynonymous polymorphisms, 3 were predicted to result in nonconservative
amino acid substitutions. Only one of these nonconservative substitutions occurred
at above 0.10 MAF, 10629 (A140D), which occurred at 0.34 MAF in the EA population
only. Because the minimal regulatory region of hGSTO1-1 has not yet been
characterized, we cannot speculate as to which polymorphisms could be occurring
in regulatory regions. Notwithstanding the amino acid diversity, perhaps the
most notable features of the genetic evaluation of hGSTO1-1 are the striking
lack of polymorphism in the IA group and the low complexity of the EA group.
One high-frequency polymorphism, 668, is common to both the IA group and the
EA group. Because the IA group probably derives from Asia, the appearance of
this polymorphism in both these geographically diverse groups suggests that
this may be an ancient polymorphism. Aside from polymorphism 668, the IA group
is monomorphic with respect to polymorphisms above a 0.10 MAF. The EA group
has 7 additional polymorphisms above this MAF threshold, but they are all in
a high degree of LD. This linked cluster of polymorphisms includes 1 nonsynonymous
polymorphism, 10629. Thus, for the IA group, only 1 polymorphism, 668, is necessary
to define all common haplotypes. In the EA group, only 2 polymorphisms, 668
and 1 polymorphism from the cluster of 7 linked polymorphisms, are necessary
to define all of the common haplotypes. Several factors may explain the difference
in overall variation in hGSTO1-1 between the IA and EA groups, including
demographic events or, alternatively, selection pressure on this genomic region.
Perhaps of greater significance is that for Mexican individuals that are some
admixture between EA and IA, the extent to which an individual might be polymorphic
for hGSTO1-1 is related to the degree of European admixture in his/her
ancestry. Thus, genetic association studies of hGSTO1-1 in Mexican Hispanics
should be carefully controlled for potential confounding by admixture.
To date, two studies have evaluated polymorphisms in hGSTO1-1. Tanaka-Kagawa
et al. (2003), using polymorphism data from the Single Nucleotide Polymorphism
database (dbSNP; http://www.ncbi.nlm.nih.gov/SNP/)
studied 2 polymorphisms that were predicted to result in nonsynonymous changes,
A140D and T217N. Substrate-dependent alterations in the resultant polymorphic
proteins were observed. No validation of the presence or frequency of these
2 polymorphisms in human subjects was performed. Recently, Whitbread et al (2003).
reported functional characterization of hGSTO1-1, together with polymorphism
screening and validation in human subjects of three ancestries, African, Australian
(EA), and Chinese. The authors based their polymorphism screening on existing
polymorphisms in several databases. Through successive tiers of validation,
only 1 of 26 hGSTO1-1 polymorphisms originally found in the databases
was observed to occur in any of the three ethnic groups. This polymorphism resulted
in a predicted nonsynonymous amino acid substitution, A140D. In the course of
the study, the authors also discovered an insertion/deletion polymorphism that
caused a deletion of residue E155 (E155del). Finally, the authors generated
expression constructs for the three observed haplotypes of these two polymorphisms
and assayed the resultant in vitro expressed protein function in enzymatic
assays. Their functional analysis demonstrated altered thiol transferase and
glutathione conjugation for the A140, E155del haplotype. Our study also identified
A140D (10629) and E155del (10674), and we discovered 1 additional nonsynonymous
polymorphism in EA subjects, E208K (14902), and 1 in IA subjects, A236V (14987).
The Whitbread study (Whitbread et al. 2003) illustrates two commonly encountered
limitations of in silico-based polymorphism screening, namely, lack of
validation of database polymorphisms and incomplete characterization of the
gamut of commonly occurring polymorphisms in the population. In this regard,
it is important to note that, of our 22 EA subjects, the same two subjects that
were heterozygous for E155del, were also heterozygous for E208K. Thus, it is
possible that these 2 polymorphisms are in substantial LD in EA subjects. As
a result, it is possible that, by testing the 155 deletion, in the absence of
the linked E208K substitution (an A140, E155del protein vs. an A140, E155del,
E208K protein) the expression constructs in the Whitbread study do not accurately
represent the commonly encountered hGSTO1-1 proteins, at least in their EA Australian
group. This is particularly significant in light of the nature of the predicted
E208K substitution, in which an acidic amino acid is substituted by a basic
amino acid. Further testing is necessary to determine if these polymorphisms
occur together in other ethnic groups.
Along with the EA and IA groups, we sequenced both hNP and hGSTO1-1
in one chimpanzee DNA sample (data not shown). Chimpanzees, the closest nonextinct
primate relative of humans, do not biotransform arsenic into methylated species
but do demonstrate arsenate reductase activity (Vahter et al. 1995; Wildfang
et al. 2001). Thus, it was not surprising that we observed a high degree of
protein homology between humans and chimpanzees in hNP and hGSTO1-1,
with only one amino acid difference between human and chimpanzee hGSTO1-1,
a conservative substitution of isoleucine (human) for valine (chimp) at residue
26. Two amino acid differences were observed in hNP. At residue 51, a
site where we observed a glycine to serine nonsynonymous polymorphism in the
human subjects, the chimp DNA sequence predicted a serine residue. At residue
277, all of our subjects were predicted to code for isoleucine, whereas the
chimp coded for valine.
These data provide a functionally annotated catalog of commonly occurring
genetic polymorphisms, in both protein coding and potential gene regulatory
regions, in two important xenobiotic-metabolizing genes in populations that
make up the genetic background of a substantial portion of Europe and the Americas.
The combination of functional polymorphisms, clusters of linked polymorphisms,
and haplotypes provide an essential framework from which to design genetic association
studies to test key phenotypes related to arsenic biotransformation, such as
urinary arsenic metabolic profile and susceptibility to arsenic-induced disease. |
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