PMCCPMCCPMCC

Search tips
Search criteria 

Advanced

 
Logo of iaiPermissionsJournals.ASM.orgJournalIAI ArticleJournal InfoAuthorsReviewers
 
Infect Immun. Dec 2002; 70(12): 6919–6925.
PMCID: PMC133071
Association between the Tumor Necrosis Factor Locus and the Clinical Outcome of Leishmania chagasi Infection
Theresa M. Karplus,1 Selma M. B. Jeronimo,2 Haeok Chang,1 Bethany K. Helms,1 Trudy L. Burns,3 Jeffrey C. Murray,4 Adele A. Mitchell,5 Elizabeth W. Pugh,5 Regina F. S. Braz,6 Fabiana L. Bezerra,6 and Mary E. Wilson1,7,8*
Departments of Internal Medicine,1 Departments of Biochemistry,2 Biostatistics,3 Pediatrics, University of Iowa,4 Center for Inherited Diseases Research, Johns Hopkins University, Baltimore, Maryland,5 Microbiology, Universidade Federal do Rio Grande do Norte, Natal, RN, Brazil,6 Microbiology,7 Veterans Affairs Medical Center, Iowa City, Iowa8
*Corresponding author. Mailing address: Department of Internal Medicine, University of Iowa, SW34-GH, Iowa City, IA 52242. Phone: (319) 356-3169. Fax: (319) 356-4600. E-mail: mary-wilson/at/uiowa.edu.
Present address: Vancouver Clinic, Vancouver, Wash.
Present address: School of Medicine, Johns Hopkins University, Baltimore, Md.
Received June 18, 2002; Revised July 30, 2002; Accepted September 15, 2002.
A periurban outbreak of visceral leishmaniasis (VL) caused by the protozoan Leishmania chagasi is ongoing outside Natal, northeast Brazil. Manifestations range from asymptomatic infection to disseminated visceral disease. Literature reports suggest that both genetic and environmental factors influence the outcome of infection. Due to the association of the tumor necrosis factor (TNF) locus with other infectious diseases, we examined whether polymorphic alleles at this locus are associated with the outcome of L. chagasi infection. Neighborhoods with ongoing transmission were identified through patients admitted to local hospitals. Altogether, 1,024 individuals from 183 families were classified with the following disease phenotypes: (i) symptomatic VL, (ii) asymptomatic infection (positive delayed-type hypersensitivity [DTH+]), or (iii) no evidence of infection (DTH−). Genotypes were determined at a microsatellite marker (MSM) upstream of the TNFB gene encoding TNF-β and at a restriction fragment length polymorphism (RFLP) at position −307 in the promoter of the TNFA gene encoding TNF-α. Analyses showed that the distribution of TNFA RFLP alleles (TNF1 and TNF2) and the TNF MSM alleles (TNFa1 to TNFa15) differed between individuals with VL and those with DTH+ phenotypes. TNF1 was transmitted more frequently than expected from heterozygous parents to DTH+ offspring (P = 0.0006), and haplotypes containing TNF2 were associated with symptomatic VL (P = 0.0265, transmission disequilibrium test). Resting serum TNF-α levels were higher in TNF1/2 heterozygotes than in TNF1/1 homozygotes (P < 0.05). These data led us to hypothesize that an individual's genotype at the TNF locus may be associated with whether he or she develops asymptomatic or symptomatic disease after L. chagasi infection. The results preliminarily suggest that this may be the case, and follow-up with larger populations is needed for verification.
The Leishmania spp. are obligate intracellular protozoa that cause a spectrum of diseases, including cutaneous, mucocutaneous, and visceral leishmaniasis (VL), in tropical or subtropical countries. In Latin America, the form of leishmaniasis leading to most fatalities, VL, is caused by Leishmania chagasi (44). The outcome of L. chagasi infection ranges in severity from asymptomatic infection to a severe progressive wasting disease called VL, which has 10% mortality even with medical treatment (5, 33, 34, 44). The factors that determine whether an individual will develop asymptomatic or symptomatic disease after L. chagasi infection are not defined.
Malnutrition, young age, and gender in those over age 10 predispose individuals to develop VL (21, 31). In addition, studies of inbred mice have led investigators to hypothesize that genetic factors may also contribute to the outcome of human disease (10, 12). Supporting this hypothesis, several groups of researchers have independently documented familial aggregation of either symptomatic VL or positive delayed-type hypersensitivity (DTH) to leishmania antigen, a measure of asymptomatic infection (1, 12, 19, 28, 34). The results of segregation analysis of symptomatic VL in multicase families from northern Brazil were consistent with the hypothesis that susceptibility to active disease is influenced by an additive dominant single gene (11). As reported in a previous study, comparison of siblings of VL patients with the general population showed that the sibling relative risk for VL was 33.6 (43). The results of a second segregation analysis of individuals with positive DTH skin test reactivity to leishmania antigen in families from a region where leishmaniasis is endemic were also consistent with the hypothesis that genetic factors contribute to asymptomatic L. chagasi infection in Brazilians; the data were consistent with a contribution from a recessive or additive gene(s) (28). These data led us to hypothesize that an individual's genetic makeup may determine in part how he or she will respond to L. chagasi infection.
Leishmaniasis is a vector-borne disease transmitted by Phlebotomus or Lutzomyia sp. sand flies, insects with a short flight pattern and focal habitat (44, 63). Identification of humans who are exposed is difficult with such a vector-borne disease. A periurban outbreak of VL outside the city of Natal, northeast Brazil, allowed us to identify neighborhoods in which there was recent or ongoing transmission of L. chagasi infection. Unlike prior studies which have focused on either patients with VL or individuals with asymptomatic infection (positive skin test result for DTH to leishmania antigen), our study differentiated among individuals with active disease, individuals with asymptomatic infection, and individuals living in households with a high chance of exposure but who remained disease free. The tumor necrosis factor (TNF) locus, which includes genes encoding TNF-α and TNF-β, has been associated with the outcome of several infectious diseases, including malaria and mucosal leishmaniasis (20, 24, 29, 40, 56, 58). In addition, VL is accompanied by high levels of TNF-α (6). The purpose of the present study was to assess the contribution of polymorphic markers at the TNF locus to the different clinical outcomes of L. chagasi infection.
Study design.
Individuals with active VL were identified after admission to one of three public hospitals in Natal. Criteria for a diagnosis of VL included symptoms of leishmaniasis, a clinical response to antimony therapy, and either a bone marrow smear containing leishmania amastigotes or a positive serologic reaction to total leishmania and k39 antigens (52). Diagnoses of VL were confirmed through hospital records. Families of patients and families living in adjacent households (neighborhood families) were enrolled in the study. Neighborhood families were chosen by selection of the household containing a nuclear family with children that was living nearest to the index family. The neighborhood families were excluded prior to recruitment if they lived more than 500 m away. Most neighboring families lived between 2 and 10 m away from index families. If two neighboring families lived equally close to the dwelling of the VL index family, then more than one neighborhood family was enrolled for that particular index family.
After obtaining informed consent, family members were interviewed in a group setting to determine exposure, medical history, and family pedigree. Subjects underwent a physical examination. Blood was drawn for complete blood count, white blood cell differential count, leishmania serology testing, and DNA extraction. A Montenegro (L. chagasi antigen) DTH skin test (kindly provided by Steven Reed, Infectious Diseases Research Institute, Seattle, Wash.) was performed. An area of induration of ≥5 mm at 48 to 72 h after testing was considered a positive result. Any medical conditions discovered, including symptoms and serology suggesting VL, were treated or referred for appropriate medical care.
Subjects and pedigrees.
Phenotypes and genotypes were determined for 1,024 individuals from 183 families. Eighty-three families were selected because one or more members had a case of VL; 100 families were neighborhood families. Of the 183 families, 85 contained a member with current VL or a history of VL and 98 had no members with VL. Family size ranged from 1 to 27 members (mean, 6.9). Disease phenotypes were defined as follows: (i) VL, active or prior VL (104 individuals); (ii) DTH+, asymptomatic infection indicated by a positive Montenegro skin test result but without a history of VL (381 individuals); and (iii) DTH−, negative leishmania serology and a negative Montenegro test result but presumably exposed to VL due to residence for ≥4 years in or near households where individuals had acquired VL (513 individuals). Twenty-six individuals with positive serology but negative Montenegro test results and no history of VL were excluded from genetic studies, since seropositivity is usually transient and these individuals could resolve into any of the other phenotypes. Eighteen families had more than one case of VL; one family had three cases.
Serology was measured by using published enzyme-linked immunosorbent assay (ELISA) protocols, using both whole L. chagasi promastigote antigen and recombinant k39 (rk39; kindly provided by Steven Reed) (17, 27, 52). Briefly, 96-well ELISA plates were coated with 200 μg of L. chagasi lysate or 50 μg of rk39, followed by incubation in patient serum at a dilution of 1:500. After the blocking and washing steps, the reaction was developed with protein A-horseradish peroxidase (Boehringer Mannheim) and 2,2′-azinobis(3-ethylbenzthiazoline-6-sulfonic acid) (ABTS) as previously reported (17). ELISA plates included positive control VL patient sera and negative control sera from unexposed individuals (26). L. chagasi antigen was prepared from a local isolate of L. chagasi.
DNA was extracted from 10 ml of anticoagulated whole blood (EDTA) by erythrocyte lysis in 70 μg of NH4H2CO3/ml and 7.0 mg of NH4Cl/ml followed by lysis of leukocytes in 1% sodium dodecyl sulfate, 100 mM EDTA, and 200 mM Tris (pH 8.5) and precipitation in isopropanol.
Genotyping methods.
Genotypes were determined for the TNF dinucleotide microsatellite marker (TNF MSM), a marker located just upstream of the TNFB gene encoding TNF-β (Fig. (Fig.1)1) (61). This TNF MSM is the most polymorphic of the five microsatellites (designated TNFa to TNFe) in the TNF locus. PCR was performed on 40 ng of genomic DNA with primers TNFB.IR2 (5′-GCCCTCTAGATTTCATCCAGCCACA-3′) and TNFB.IR4 (5′-CCTCTCTCCCCTGCAACACACA-3′) (GDB:574102; Integrated DNA Technologies, Iowa City, Iowa) (42). Fifteen alleles of 101 to 125 bp containing CA repeats, which were detected by silver staining of 6% denaturing polyacrylamide gels, corresponded to the reported TNFa1 to TNFa15 alleles (30, 35).
FIG. 1.
FIG. 1.
Map of the human TNF locus and HLA loci based upon the studies of Wilson et al. (61) and Zanelli et al. (64). The drawing indicates the relative positions of the TNFA and TNFB genes encoding TNF-α and TNF-β, respectively, with respect (more ...)
TNF-α −307 promoter polymorphism.
We evaluated a restriction fragment length polymorphism (RFLP) reported at position −307 in the promoter of the TNFA gene encoding TNF-α (20) (Fig. (Fig.1).1). A 107-bp fragment of DNA was amplified using primer pairs 5′-AGGCAATAGGTTTTGAGGGCCAT-3′ and 5′-TCCTCCCTGCTCCGATTCCG-3′ (GDB:196368). Digestion of the TNF1 (−307*G) allele with NcoI yielded fragments of 87 and 20 bp on a 3% agarose gel, whereas TNF2 (−307*A) remained uncut (107 bp) (30, 60). For RFLP analysis, 751 individuals were chosen because they could be included in the transmission disequilibrium test (TDT) or case-control analyses.
HLA region markers.
MSMs near the flanking major histocompatibility complex (MHC) class II (between TNFA and HLA-DR) and MHC class I (located telomeric to HLA-B) regions were evaluated (Fig. (Fig.1).1). The trinucleotide repeat marker D6S1014 (CHLC.GCT4B05) between the HLA-DR region and HSP70-2 was amplified using primers 5′-GGGTCTGACCACTGAGACAC-3′ and 5′-CAGTGAGAGCTCTGAGGGTC-3′. The Cooperative Human Linkage Center (CHLC) marker GATA43E06 (D6S2260) located telomeric to HLA-B was amplified using primers 5′-TCTGTATACTTTCCCTGCAGG-3′ and 5′-CCTGGGCTTAAGAAAGCTTT-3′ (64). The dinucleotide repeat marker D6S1666 (AFMc019yc5) located 0.25 Mb telomeric to the HLA-A region was amplified with primers 5′-CTGAGTTGGGCAGCATTTG-3′ and 5′-ACCCAGCATTTTGGAGTTG-3′.
TNF ELISA.
TNF-α in the serum was detected by ELISA. The reagents used were 4 μg of monoclonal antibody MAB610/ml (capture), 200 ng of biotinylated BAF210 goat antiserum/ml (detection), streptavidin horseradish peroxidase (Zymed Laboratories, San Francisco, Calif.), and ABTS developing reagent (Kirkegaard & Perry Laboratories, Gaithersburg, Md.). A standard curve was generated with recombinant human TNF-α (R&D Systems, Minneapolis, Minn.). The sensitivity was 5 pg/ml.
Statistical analyses.
Allele frequencies were estimated using unrelated individuals from different pedigrees (excluding probands) or within pedigrees when related only by marriage (Table (Table1).1). The association between genetic markers and case-control status, with different definitions of “case” and “control” as shown in Table Table2,2, was investigated using contingency table analysis as implemented in the CLUMP program (51). This program compares the frequency of each allele for a particular phenotype with the frequency of all other alleles clumped together. Monte Carlo simulations were conducted with the CLUMP program to determine asymptotic P values that account for sparse cells in contingency tables. The T3 test statistic reported here resulted from the identification of a single allele which, when compared to all other alleles clumped together, provided a two-by-two table with the largest chi-square statistic (lowest P value) for the data.
TABLE 1.
TABLE 1.
TNF MSM and TNF-α promoter RFLP allele frequencies
TABLE 2.
TABLE 2.
Case-control analyses of the distribution of alleles in unrelated individuals with different phenotypes
An extended TDT for multiallele marker loci was used as implemented in the ETDT program (50). This method evaluates the pattern of allele transmission across genotypes by using logistic regression. The program considers all alleles across families, so that only alleles preferentially transmitted to multiple affected children are significant. Only unrelated trios were included in the analysis. In some cases, this exceeded the total number of pedigrees when nuclear families were connected by marriage. Haplotypes were determined by examination of three-generation families in which it was evident which TNF MSM and TNF-α alleles were syntenic. The extended TDT was also used to assess disequilibrium in the transmission of these 30 haplotypes.
SIMLINK was used to estimate the power to detect linkage in these families (14).
Allele frequencies.
Microsatellite amplification identified 15 different TNF MSM alleles in 1,024 individuals (Table (Table1).1). The 751 individuals that could be included in association analyses were also genotyped for the −307 polymorphism in the TNFA promoter (TNF1 and TNF2). It was found that 596 individuals were homozygous for TNF1 (72%), 216 were heterozygous (TNF1/2; 26%), and 18 were homozygous for TNF2 (2%). The frequency of the less common TNF2 allele was 0.152, similar to that of other populations (20, 40, 46, 59, 61). The distribution of the TNF MSM alleles and the distribution of TNF-α alleles were consistent with a Hardy-Weinberg equilibrium. This was true both when all individuals were considered in the analysis and when only unrelated individuals were included.
The TNF MSM polymorphism and the TNFA promoter RFLP are only 3 kb apart from each other on chromosome 6p. As expected, these markers are tightly associated in linkage disequilibrium (P = 0.0007, chi-square test). TNF2 occurred relatively more frequently among individuals bearing the TNFa5 allele (32.4%). In contrast, TNF2 occurred less frequently among individuals bearing the TNFa11 or TNFa13 allele (9.3 and 5.0%, respectively).
Case-control analyses.
There were differences in the distributions of the TNF MSM and TNFA promoter RFLP alleles between unrelated individuals in the different phenotype groups (Table (Table2).2). TNFa5 was more common in VL patients than in DTH+ individuals, whereas TNFa11 and TNFa13 were more common in DTH+ individuals than in those with other phenotypes. The TNFA promoter RFLP allele TNF2 occurred more frequently in VL patients (17.1%) than in DTH+ (6.3%) individuals.
ETDT.
A TDT (ETDT program) was used to assess the pattern of transmission of TNFA promoter RFLP alleles and the 15 TNF MSM alleles from heterozygous parents to their offspring with either the VL or DTH+ phenotype (50). Only unrelated trios were included in the analysis. The results indicated an excess frequency of transmission of specific alleles at each locus (Tables (Tables33 and and4).4). Notably, TNF1 was passed 28 of 36 times from heterozygous parents to DTH+ offspring (P = 0.0006) compared with 38 of 84 times to DTH− offspring (P = 0.3824) (Table (Table4).4). This suggests an association between TNF1 and the tendency to develop asymptomatic infection. TDT results for passage of TNFA promoter RFLP alleles to VL offspring did not meet statistical significance, possibly because of an insufficient number of trios with heterozygous parents (n = 25). Nonetheless, ETDT analysis of the transmission of TNF MSM/TNFA RFLP haplotypes, which include 30 alleles, to VL offspring yielded a P value of 0.027 (n = 59 trios).
TABLE 3.
TABLE 3.
Transmission disequilibrium analysis of the association of TNF MSM (15 alleles) and TNFA promoter RFLP (2 alleles) with the three phenotypesa
TABLE 4.
TABLE 4.
Frequencies with which TNFA promoter alleles were passed from heterozygous parents to offspring with the different phenotypes in unrelated trios
Power studies.
With VL defined as affected, DTH+ defined as unaffected, and DTH− defined as unknown, SIMLINK analysis of the families with two or more cases of VL (14) indicated that the power of finding a lod score of >1.0 for these families was 0.46 at a θ value of 0.0 or 0.23 at a θ value of 0.10. This result suggested that we had little power to detect linkage to a susceptibility gene by using linkage methods of analysis. This was not a surprise since a simple Mendelian model of inheritance must be designated to perform nonparametric linkage, and such a model is not appropriate for this complex disease. Therefore, we relied upon association methods as the most appropriate method of analysis for this population.
ETDT and case-control analysis of HLA-DR and HLA-B markers.
Because the TNF locus is in linkage disequilibrium with HLA, it is possible that the low P values resulting from the TDT analysis were actually due to strong linkage disequilibrium with nearby HLA genes. We therefore determined the genotype by using markers in flanking regions toward both the class II and class I HLA regions. Case-control and TDT analyses were performed on the same trios used above for analysis of the VL and DTH+ phenotypes (Table (Table5).5). Six alleles were detected at the D6S1014 marker between HLA-DR and HSP70-2, which in turn lies between HLA-DR and the TNF locus (Fig. (Fig.1).1). Five alleles were detected at the D6S2260 marker that lies telomeric to HLA-B. Thirteen alleles were detected at the D6S1666 (AFMc019yc5) marker which is further in the direction of the telomere, near HLA-A. The results of case-control comparisons (CLUMP program) were not significant for any of the phenotypic comparisons with these markers. TDT analysis (ETDT program) of the D6S2260 marker nearest to HLA-B yielded high (nonsignificant) P values as well. However, analysis of the D6S1014 marker (near HLA-DR) in DTH+ trios by using ETDT yielded a P value of 0.0223, in contrast to a value of 0.6110 for VL trios. Analysis of the D6S1666 marker (telomeric to HLA-A) that lies further from the TNF locus in VL trios yielded a P value of 0.0201 compared with a value of 0.2271 for DTH+ trios. Further studies are needed to verify whether there is an association between the DTH+ phenotype and the HLA-DR marker as well as an association between the VL phenotype and markers near HLA-A.
TABLE 5.
TABLE 5.
Case-control (CLUMP program) and ETDT analysis of microsatellites in the HLA-DR (D6S1666) and HLA-B (D6S2260) regions
Serum TNF-α levels.
Sera were drawn at the time of study entry. TNF-α levels were determined for all individuals for whom there were remaining serum samples after leishmania serology testing. Basal serum levels of TNF-α, measured by ELISA, for individuals with different TNFA promoter RFLP genotypes were compared. Attempts were made to include only individuals who were healthy, since TNF-α may transiently rise during acute illness.
There is an increase in TNF-α during active VL (6). Our VL group included individuals at different stages of treatment as well as those cured of prior infection. Furthermore, we had serum from only a subset of VL individuals, in whom the TNF-α serum levels were as follows: 124 ± 121 pg/ml (mean ± standard deviation) for TNF1/1 individuals (n = 4; values, 0, 0, 487, and 10); 31 ± 19 pg/ml for TNF1/2 individuals (n = 10); and 47 pg/ml for TNF2/2 individuals (n = 1). The extreme variability in TNF-α serum levels among VL patients was likely due to the small number of samples and the varied times at which serum was drawn with respect to treatment. Since there was no way to correct for these parameters, we excluded the VL group from the overall statistical analysis shown in Table Table6.6. Including healthy persons only, therefore, individuals with the TNF1/1 genotype had significantly lower levels of TNF-α than did TNF1/2 heterozygotes (Table (Table66).
TABLE 6.
TABLE 6.
Serum TNF-α levels in DTH+ or DTH− individuals with different genotypes
Recent literature includes many reports of genetic factors that influence the outcome of human infection with intracellular pathogens such as Mycobacterium spp., Salmonella spp., and Plasmodium falciparum (3, 4, 7, 8, 25, 36, 40, 48, 57). Familial aggregation studies and segregation analyses have also suggested that genetic factors contribute to the outcome of human VL (10-13, 28). In the present study, we investigated whether genetic variability at or near the TNF locus is associated with the development of symptomatic or asymptomatic L. chagasi infection. This study was unique in that we were able to differentiate symptomatic from asymptomatic infection in individuals living in neighborhoods where there was ongoing transmission of L. chagasi. The TNF locus was studied as a candidate susceptibility gene locus for three reasons. First, TNF-α levels are elevated in acute VL (6). Second, polymorphisms at the TNF locus have been associated with a large number of autoimmune and some infectious diseases (24, 29, 40, 56, 58). Third, a case-control study of 46 patients with mucocutaneous leishmaniasis, a hyperergic disease most often caused by L. braziliensis, suggested an association with the TNF2 allele (20). Visceral and mucocutaneous leishmaniasis lie at opposite poles of the spectrum of leishmaniasis. Immune responses are suppressed and the parasite load is high during VL, whereas there are few parasites but a vigorous immune response during mucocutaneous leishmaniasis. We hypothesized that distinct and opposite immune factors may predispose individuals to develop each of these diseases. However, our results suggested that the same genotype at the TNF locus is associated with development of these contrasting forms of disease.
Analysis of 1,024 subjects living in neighborhoods where leishmaniasis is endemic suggested an association between the outcome of L. chagasi infection and alleles at the TNF locus. The strongest association was found between asymptomatic infection (DTH+) and a polymorphism in the TNF-α promoter at position −307 with respect to the transcription start site (erroneously labeled −308 in the literature [62]). The CA repeat at the TNF MSM was also associated with the DTH+ phenotype although not as strongly. There was not complete association between the two markers that we tested. This could be due to historical recombination between the two markers, although it is more likely that there have been mutations of the CA repeats since they lie in noncoding regions of the genome. Analysis of extended haplotypes, considering genotypes at both the TNF MSM and the TNF-α RFLP markers, also suggested an association between TNF alleles and symptomatic VL. According to the results of case-control analysis, the genetic differences were greatest between individuals with symptomatic and those with asymptomatic L. chagasi infection (VL versus DTH+). Due to the use of multiple testing in this study (multiple markers, phenotypes, and analytical methods), the chance of a type I error was increased. As the most significant P values (0.0006 for TDT) were greater than the value of 0.0001 expected of a genome-wide linkage scan, the results must be regarded as preliminary but suggestive that further study with larger populations is worthwhile. Furthermore, due to the smaller number of VL cases compared with cases of asymptomatic infection, the association between TNF and VL warrants further studies with a larger sample size.
Analysis of the same population by using MSMs in the HLA-B and HLA-DR regions did not reveal as strong an association as that with TNF, and there was a lack of association with the marker nearest to HLA-B. The lowest P values were obtained in association analyses of asymptomatic infection (DTH+) with the D6S1014 marker near HLA-DR (P = 0.022) or in analyses of symptomatic disease (VL) with the D6S1666 marker telomeric to HLA-A (P = 0.020). The negative results for an association between the D6S1666 marker and disease suggest that the TNF locus association results are probably not caused by a stronger association with MHC class I genes. The P values for the D6S1014 marker and DTH+ phenotype warrant follow-up, but again, these data are weaker rather than stronger than the data for an association of TNF with asymptomatic disease. Taken together, these analyses favor a model in which TNF1 is associated with the development of asymptomatic L. chagasi infection detectable by a positive Montenegro skin test exam, independent of a possible association with MHC class I and class II genes.
A case-control study with Gambian children suggested that TNF2/2 homozygotes had a sevenfold increased risk of death or neurological sequelae from malaria than did heterozygotes (40). A previous study of individuals with or without VL in Belém, northern Brazil, did not document linkage with the TNF locus (12). However, by distinguishing those with active VL from those with asymptomatic infection and by distinguishing each of these from the population that is DTH− but likely exposed, we were able to detect an association that might have been inapparent when disease-negative individuals were analyzed as a single group.
Numerous polymorphisms at the TNFA locus have been reported, with conflicting reports of functional significance. Promoter polymorphisms cluster in repeating 4-base G/A motifs (49). Whereas some studies show that the −307 promoter polymorphism influences the amount of TNF-α produced by stimulated peripheral blood mononuclear cells (15, 39), others suggest that there is no effect (24, 32, 41, 47). Whether the results are significant depends in part upon the number of subjects examined and the stimulus chosen (2). Studies using reporter genes under the control of the TNF-α promoter have also produced conflicting results (16, 18, 38, 53, 55, 62), which differ depending on the length of the 5′ untranslated region used and whether a 3′ untranslated region was cloned adjacent to the reporter gene (2). Those studies that have reported a difference in expression, whether or not the difference reached statistical significance, have consistently shown that transcription and/or TNF-α levels are increased in individuals with the rarer −307*A (TNF2) allele. Consistently, TNF1/1 homozygotes in the population we studied had significantly lower basal TNF-α serum levels than did TNF1/2 heterozygotes. It is possible that this result was due to a sequence tightly linked to the −307 polymorphism. Nonetheless, the data suggest that a polymorphic sequence(s) at or near the −307 locus influences TNF-α levels and disease outcome.
The data discussed above led us to hypothesize that the propensity of an individual to develop asymptomatic infection versus symptomatic disease after infection with L. chagasi is associated in part with his or her genotype at the TNF locus. If this hypothesis is true, then the symptoms of VL would be due in part to the level of TNF-α achieved (6, 22, 45, 54). Moderate levels of TNF-α, as would be expected among TNF1 homozygotes, would facilitate control of intracellular infection. Higher levels of TNF-α in individuals bearing the TNF2 allele would predispose them to clinical manifestations of VL including fever, wasting, anorexia, pancytopenia, and polyclonal B-cell activation (6, 9). Among persons infected with Plasmodium falciparum, the TNF2 allele is found more frequently in individuals who developed the severe cerebral form of disease (40). In an analogous manner, our hypothesis would indicate that heterozygotes in our study population who harbor the TNF2 allele are more likely to develop the severest visceral form of disease after exposure to L. chagasi rather than asymptomatic or limited infection. The above-mentioned data do not distinguish whether the TNFA RFLP is a functional polymorphism or whether it is in linkage disequilibrium with a true functional polymorphism. Nonetheless, they do lead to the hypothesis that genetically determined high-level TNF-α responses to L. chagasi infection might predispose individuals, in part, to development of the severest visceral form of disease due to this intracellular protozoan. It may be reasonable to study agents that can lower TNF-α levels, such as thalidomide or pentoxifylline, as adjuvants to therapy for VL (23, 37).
Acknowledgments
This study was supported in part by a Tropical Medicine Research Center grant and other grants from the National Institutes of Health (AI-30639-08, DK/AI2550, AI32135, and TW01369-01), a grant from the Conselho Nacional de Pesquisa (S.M.B.J.), NIH training grant T32 AI07511 (T.M.K.), a VA Merit Review grant (M.E.W.), CIDR contract N01-HG-65403 (E.W.P.), and a pilot grant from the University of Iowa Howard Hughes institutional grant.
Notes
Editor: W. A. Petri, Jr.
1. Alcais, A., L. Abel, C. David, M. E. Torrez, P. Flandre, and J. P. Dedet. 1997. Evidence for a major gene controlling susceptibility to tegumentary leishmaniasis in a recently exposed Bolivian population. Am. J. Hum. Genet. 61:968-979. [PubMed]
2. Allen, R. D. 1999. Polymorphism of the human TNF-α promoter—random variation or functional diversity? Mol. Immunol. 36:1017-1027. [PubMed]
3. Altare, F., A. Durandy, D. Lammas, J.-F. Emile, S. Lamhamedi, F. Le Deist, P. Drysdale, E. Jouanguy, R. Doffinger, F. Bernaudin, O. Jeppsson, J. A. Gollob, E. Meinl, A. W. Segal, A. Fischer, D. Kumararatne, and J.-L. Casanova. 1998. Impairment of mycobacterial immunity in human interleukin-12 receptor deficiency. Science 280:1432-1435. [PubMed]
4. Altare, F., D. Lammas, P. Revy, E. Jouanguy, R. Doffinger, S. Lamhamedi, P. Drysdale, D. Scheel-Toellner, J. Girdlestone, and P. Darbyshire. 1998. Inherited interleukin 12 deficiency in a child with bacille Calmette-Guérin and Salmonella enteritidis disseminated infection. J. Clin. Investig. 102:2035-2040. [PMC free article] [PubMed]
5. Badaro, R., T. C. Jones, E. M. Carvalho, D. Sampaio, S. G. Reed, A. Barral, R. Teixeira, and W. D. Johnson, Jr. 1986. New perspectives on a subclinical form of visceral leishmaniasis. J. Infect. Dis. 154:1003-1011. [PubMed]
6. Barral-Netto, M., R. Badaro, A. Barral, R. P. Almeida, S. B. Santos, F. Badaro, D. Pedral-Sampaio, E. M. Carvalho, E. Falcoff, and R. Falcoff. 1991. Tumor necrosis factor (cachectin) in human visceral leishmaniasis. J. Infect. Dis. 163:853-857. [PubMed]
7. Bellamy, R., C. Ruwende, T. Corrah, K. P. McAdam, H. C. Whittle, and A. V. Hill. 1999. Tuberculosis and chronic hepatitis B virus infection in Africans and variation in the vitamin D receptor gene. J. Infect. Dis. 179:721-724. [PubMed]
8. Bellamy, R., C. Ruwende, T. Corrah, K. P. McAdam, H. C. Whittle, and A. V. S. Hill. 1998. Variations in the NRAMP1 gene and susceptibility to tuberculosis in West Africans. N. Engl. J. Med. 338:640-644. [PubMed]
9. Beutler, B. A. 1999. The role of tumor necrosis factor in health and disease. J. Rheumatol. 26(Suppl. 57):16-21. [PubMed]
10. Blackwell, J. M. 1996. Genetic susceptibility to leishmanial infections: studies in mice and man. Parasitology 112:S67-S74. [PubMed]
11. Blackwell, J. M. 1998. Genetics of host resistance and susceptibility to intramacrophage pathogens: a study of multicase families of tuberculosis, leprosy and leishmaniasis in northeastern Brazil. Int. J. Parasitol. 28:21-28. [PubMed]
12. Blackwell, J. M., G. F. Black, C. S. Peacock, E. N. Miller, D. Sibthorpe, D. Gnananandha, J. J. Shaw, F. Silveira, Z. Lins-Lainson, F. Ramos, A. Collins, and M.-A. Shaw. 1997. Immunogenetics of leishmanial and mycobacterial infections: the Belem family study. Philos. Trans. R. Soc. Lond. B Biol. Sci. 352:1331-1345. [PMC free article] [PubMed]
13. Blackwell, J. M., G. F. Black, C. Sharples, S.-S. Soo, C. S. Peacock, and N. E. Miller. 1999. Roles of Nramp1, HLA, and the gene(s) in allelic association with IL-4, in determining T helper subset differentiation. Microbes Infect. 1:95-102. [PubMed]
14. Bloughman, L. M., and M. Boehnke. 1989. Estimating the power for a proposed linkage study for a complex genetic trait. Am. J. Hum. Genet. 44:543-551. [PubMed]
15. Bouma, G., J. B. A. Crusius, M. O. Pool, J. J. Kolkman, B. M. E. Von Blomberg, P. J. Kostense, M. J. Giphart, G. M. T. Schreuder, S. G. M. Meuwissen, and A. S. Pena. 1996. Secretion of tumour necrosis factor α and lymphotoxin α in relation to polymorphisms in the TNF genes and HLA-DR alleles. Relevance for inflammatory bowel disease. Scand. J. Immunol. 43:456-463. [PubMed]
16. Braun, N., U. Michel, B. P. Ernst, R. Metzner, A. Bitsch, F. Weber, and P. Reickman. 1996. Gene polymorphism at position −308 of the tumor necrosis factor-α (TNF-α) in multiple sclerosis and its influence on the regulation of TNF-α production. Neurosci. Lett. 215:75-78. [PubMed]
17. Braz, R. F. S., E. T. Nascimento, D. R. A. Martins, M. E. Wilson, R. D. Pearson, S. G. Reed, and S. M. B. Jeronimo. The sensitivity and specificity of Leishmania chagasi recombinant K39 antigen in the diagnosis of American visceral leishmaniasis and in differentiating active from subclinical infection. Am. J. Trop. Med. Hyg., in press. [PubMed]
18. Brinkman, B. M. N., D. Zuijdgeest, E. L. Kaijzel, F. C. Breedveld, and C. L. Verweij. 1996. Relevance of the tumor necrosis factor alpha (TNFα) −308 promoter polymorphism in TNFα gene regulation. J. Inflamm. 46:32-41. [PubMed]
19. Cabello, P. H., A. M. Lima, E. S. Azevedo, and H. Krieger. 1995. Familial aggregation of Leishmania chagasi infection in northeastern Brazil. Am. J. Trop. Med. Hyg. 52:364-365. [PubMed]
20. Cabrera, M., M. A. Shaw, C. Sharples, H. Williams, M. Castes, J. Convit, and J. M. Blackwell. 1995. Polymorphism in tumor necrosis factor genes associated with mucocutaneous leishmaniasis. J. Exp. Med. 182:1259-1264. [PMC free article] [PubMed]
21. Cerf, B. J., T. C. Jones, R. Badaro, D. Sampaio, R. Teixeira, and W. D. Johnson, Jr. 1987. Malnutrition as a risk factor for severe visceral leishmaniasis. J. Infect. Dis. 156:1030-1033. [PubMed]
22. Chiofalo, M. S., D. Delfino, G. Mancuso, E. La Tassa, P. Mastroeni, and D. Iannello. 1992. Induction of tumor necrosis factor α by Leishmania infantum in murine macrophages from different inbred mice strains. Microb. Pathog. 12:9-17. [PubMed]
23. Corral, L. G. and G. Kaplan. 1999. Immunomodulation by thalidomide and thalidomide analogues. Ann. Rheum. Dis. 58(Suppl. 1):I107-I113. [PMC free article] [PubMed]
24. Danis, V. A., M. Millington, V. Hyland, R. Lawford, Q. Huang, and D. Grennan. 1994. Increased frequency of the uncommon allele of the tumour necrosis factor alpha gene polymorphism in rheumatoid arthritis and systemic lupus erythematosus. Dis. Markers 12:127-133. [PubMed]
25. de Jong, R., F. Altare, I.-A. Haagen, D. G. Elferink, T. de Boer, P. J. C. van Breda Vriesman, P. J. Kabel, J. M. T. Draaisma, J. T. van Dissel, F. P. Kroon, J.-L. Casanova, and T. H. M. Ottenhoff. 1998. Severe mycobacterial and Salmonella infections in interleukin-12 receptor-deficient patients. Science 280:1435-1438. [PubMed]
26. Evans, T. G., E. C. Krug, M. E. Wilson, A. W. Vasconcelos, J. E. de Alencar, and R. D. Pearson. 1989. Evaluation of antibody responses in American visceral leishmaniasis by ELISA and immunoblot. Mem. Inst. Oswaldo Cruz 84:157-166. [PubMed]
27. Evans, T. G., I. A. B. Vasconcelos, J. W. Lima, J. M. Teixeira, T. McAullife, U. G. Lopes, R. D. Pearson, and A. W. Vasconcelos. 1990. Canine visceral leishmaniasis in northeast Brazil: assessment of serodiagnostic methods. Am. J. Trop. Med. Hyg. 42:118-123. [PubMed]
28. Feitosa, M. F., E. Axevedo, A. M. Lima, and H. Krieger. 1999. Genetic causes involved in Leishmania chagasi infection in northeastern Brazil. Genet. Mol. Biol. 22:1-5.
29. Foster, C. B., T. Lehrnbecher, F. Mol, S. M. Steinberg, D. J. Venzon, T. J. Walsh, D. Noack, J. Rae, J. A. Winkelstein, J. T. Curnutte, and S. J. Chanock. 1998. Host defense molecule polymorphisms influence the risk for immune-mediated complications in chronic granulomatous disease. J. Clin. Investig. 102:2146-2155. [PMC free article] [PubMed]
30. Hajeer, A. H., and I. V. Hutchinson. 2000. TNF-α gene polymorphism: clinical and biological implications. Microsc. Res. Tech. 50:216-228. [PubMed]
31. Harrison, L. H., T. G. Naidu, J. S. Drew, J. E. de Alencar, and R. D. Pearson. 1986. Reciprocal relationships between undernutrition and the parasitic disease visceral leishmaniasis. Rev. Infect. Dis. 8:447-453. [PubMed]
32. Huizinga, T. W. J., R. G. L. Westendorp, E. L. Bollen, V. Keijsers, B. M. N. Brinkman, J. A. M. Langermans, F. C. Breedveld, C. L. Verweij, L. Van de Gaer, L. Dams, J. B. A. Crusuis, A. Garcia-Gonzalez, B. W. Van Oosten, C. H. Polman, and A. S. Pena. 1997. TNF-α promoter polymorphisms, production and susceptibility to multiple sclerosis in different groups of patients. J. Neuroimmunol. 72:149-153. [PubMed]
33. Jeronimo, S. M. B., R. M. Oliveira, S. Mackay, R. M. Costa, J. Sweet, E. T. Nascimento, K. G. Luz, M. Z. Fernandes, J. Jernigan, and R. D. Pearson. 1994. An urban outbreak of visceral leishmaniasis in Natal, Brazil. Trans. R. Soc. Trop. Med. Hyg. 88:386-388. [PubMed]
34. Jeronimo, S. M. B., M. J. Teixeira, A. D. Q. Sousa, P. Thielking, R. D. Pearson, and T. G. Evans. 2000. Natural history of Leishmania (Leishmania) chagasi infection in northeastern Brazil: long-term follow-up. Clin. Infect. Dis. 30:608-609. [PubMed]
35. Jongeneel, C. V., L. Briant, I. A. Udalova, A. Sevin, S. A. Nedospasov, and A. Cambon-Thomsen. 1991. Extensive genetic polymorphism in the human tumor necrosis factor region and relation to extended HLA haplotypes. Proc. Natl. Acad. Sci. USA 88:9717-9721. [PubMed]
36. Jouanguy, E., F. Altare, S. Lamhamedi, P. Revy, J.-F. Emile, M. Newport, M. Levin, S. Blanche, E. Seboun, A. Fischer, and J.-L. Casanova. 1996. Interferon-gamma-receptor deficiency in an infant with fatal bacille Calmette-Guérin infection. N. Engl. J. Med. 335:1956-1961. [PubMed]
37. Kremsner, P. G., H. Grundmann, S. Neifer, K. Sliwa, G. Sahlmuller, B. Hegenschied, and U. Bienzle. 1991. Pentoxifylline prevents murine cerebral malaria. J. Infect. Dis. 164:605-608. [PubMed]
38. Kroeger, K. M., and L. J. Abraham. 1996. Identification of an AP-2 element in the −323 to −285 region of the TNF-α gene. Biochem. Mol. Biol. Int. 40:43-51. [PubMed]
39. Louis, E., D. Franchimont, A. Piron, Y. Gevaert, N. Schaaf-Lafontaine, S. Roland, P. Mahieu, M. Malaise, D. de Groote, R. Louis, and J. Belaiche. 1998. Tumour necrosis factor (TNF) gene polymorphism influences TNF-α production in lipopolysaccharide (LPS)-stimulated whole blood cell culture in healthy humans. Clin. Exp. Immunol. 113:401-406. [PubMed]
40. McGuire, W., A. V. S. Hill, C. E. M. Allsopp, B. M. Greenwood, and D. Kwiatkowski. 1994. Variation in the TNF-α promoter region associated with susceptibility to cerebral malaria. Nature 371:508-511. [PubMed]
41. Mycko, M., W. Kowalski, M. Kwinkowski, A. C. Buenafe, B. Szymanska, E. Tronczynska, A. Plucienniczak, and K. Selmaj. 1998. Multiple sclerosis: the frequency of allelic forms of tumor necrosis factor and lymphotoxin-α. J. Neuroimmunol. 84:198-206. [PubMed]
42. Nedospasov, S. A., I. A. Udalova, and D. V. Kuprash. 1991. DNA sequence polymorphism at the human tumor necrosis factor (TNF) locus. J. Immunol. 147:1053-1059. [PubMed]
43. Peacock, C. S., A. Collins, M.-A. Shaw, F. Silveira, J. Costa, C. H. Coste, M. D. Nascimento, R. Siddiqui, J. J. Shaw, and J. M. Blackwell. 2001. Genetic epidemiology of visceral leishmaniasis in northeastern Brazil. Genet. Epidemiol. 20:383-396. [PubMed]
44. Pearson, R. D., and A. D. Q. Sousa. 1996. Clinical spectrum of leishmaniasis. Clin. Infect. Dis. 22:1-13. [PubMed]
45. Pisa, P., M. Gennene, O. Soder, T. Ottenhoff, M. Hansson, and R. Kiessling. 1990. Serum tumor necrosis factor levels and disease dissemination in leprosy and leishmaniasis. J. Infect. Dis. 161:988-991. [PubMed]
46. Pociot, F., L. Briant, C. V. Jongeneel, J. Molvig, H. Worsaae, M. Abbal, M. Thomsen, J. Nerup, and A. Cambon-Thomsen. 1993. Association of tumor necrosis factor (TNF) and class II major histocompatibility complex alleles with the secretion of TNF-α and TNF-β by human mononuclear cells: a possible link to insulin-dependent diabetes mellitus. Eur. J. Immunol. 23:224-231. [PubMed]
47. Pociot, F., A. G. Wilson, J. Nerup, and G. W. Duff. 2000. No independent association between a tumour necrosis factor-alpha promoter region polymorphism and insulin-dependent diabetes mellitus. Eur. J. Immunol. 23:3043-3049.
48. Roy, S., A. Frodsham, B. Saha, S. K. Hazra, C. G. N. Mascie-Taylor, and A. V. S. Hill. 1999. Association of vitamin D receptor genotype with leprosy type. J. Infect. Dis. 179:187-191. [PubMed]
49. Ruuls, S. R., and J. D. Sedgwick. 1999. Unlinking tumor necrosis factor biology from the major histocompatibility complex: lessons from human genetics and animal models. Am. J. Hum. Genet. 65:294-301. [PubMed]
50. Sham, P. C., and D. Curtis. 1995. An extended transmission/disequilibrium test (TDT) for multi-allele marker loci. Ann. Hum. Genet. 59:323-336. [PubMed]
51. Sham, P. C., and D. Curtis. 1998. Monte Carlo tests for associations between disease and alleles at highly polymorphic loci. Ann. Hum. Genet. 59:97-105. [PubMed]
52. Singh, S., A. Gliman-Sachs, K.-P. Chang, and S. G. Reed. 1995. Diagnostic and prognostic value of k39 recombinant antigen in Indian leishmaniasis. J. Parasitol. 8:1000-1003. [PubMed]
53. Stuber, F., I. A. Udalova, M. Book, L. N. Drutskaya, D. V. Kuprash, R. L. Turetskaya, F. U. Schade, and S. A. Nedospasov. 1996. −308 tumor necrosis factor (TNF) polymorphism is not associated with survival in severe sepsis and is unrelated to lipopolysaccharide inducibility of the human TNF promoter. J. Inflamm. 46:42-50. [PubMed]
54. Tumang, M. C. T., C. Keogh, L. L. Moldawer, D. C. Helfgott, R. Teitelbaum, J. Hariprashad, and H. W. Murray. 1994. Role and effect of TNF-α in experimental visceral leishmaniasis. J. Immunol. 153:768-775. [PubMed]
55. Uglialoro, A. M., D. Turbay, P. A. Pesavento, J. C. Delgado, F. E. McKenzie, J. G. Gribben, D. Hartl, E. J. Yunis, and A. E. Goldfeld. 1998. Identification of three new single nucleotide polymorphisms in the human tumor necrosis factor-α gene promoter. Tissue Antigens 52:359-367. [PMC free article] [PubMed]
56. Verweij, C. L. 1999. Tumor necrosis factor gene polymorphisms as severity markers in rheumatoid arthritis. Ann. Rheum. Dis. 58(Suppl. 1):120-126. [PMC free article] [PubMed]
57. Wilkinson, R. J., P. Patel, M. Llewelyn, C. S. Hirsch, G. Pasvol, G. Snounou, R. N. Davidson, and Z. Toossi. 1999. Influence of polymorphism in the genes for the interleukin (IL)-1 receptor antagonist and IL-1β on tuberculosis. J. Exp. Med. 189:1863-1873. [PMC free article] [PubMed]
58. Wilson, A. G. 1999. Genetics of tumour necrosis factor (TNF) in autoimmune liver diseases: red hot or red herring? J. Hepatol. 30:331-333. [PubMed]
59. Wilson, A. G., N. de Vries, F. Pociot, F. S. di Giovine, L. B. A. van der Putte, and G. W. Duff. 1993. An allelic polymorphism within the human tumor necrosis factor α promoter region is strongly associated with HLA A1, B8, and DR3 alleles. J. Exp. Med. 177:557-560. [PMC free article] [PubMed]
60. Wilson, A. G., F. S. di Giovine, A. I. F. Blakemore, and G. W. Duff. 1995. Single base polymorphism in the human tumour necrosis factor alpha (TNFα) gene detectable by NcoI restriction of PCR product. Hum. Mol. Genet. 1:353-357. [PubMed]
61. Wilson, A. G., F. S. di Giovine, and G. W. Duff. 1995. Genetics of tumour necrosis factor-α in autoimmune, infectious, and neoplastic diseases. J. Inflamm. 45:1-12. [PubMed]
62. Wilson, A. G., J. A. Symons, T. L. McDowell, H. O. McDevitt, and G. W. Duff. 1997. Effects of a polymorphism in the human tumor necrosis factor α promoter on transcriptional activation. Proc. Natl. Acad. Sci. USA 94:3195-3199. [PubMed]
63. Ximenes, M. F. F. M., E. G. Castellon, M. F. Souza, R. D. Pearson, M. E. Wilson, and S. M. B. Jeronimo. 2000. Distribution of Phlebotomine sandflies (Diptera: Psychodidae) in the state of Rio Grande do Norte, Brazil. J. Med. Entomol. 37:162-169. [PubMed]
64. Zanelli, E., G. Jones, M. Pascual, P. Eerligh, A. R. van der Slik, A. H. Zwinderman, W. Verduyn, G. M. T. Schreuder, E. Roovers, F. C. Breedveld, R. R. P. de Vries, J. Martin, and M. J. Giphart. 2001. The telomeric part of the HLA region predisposes to rheumatoid arthritis independently of the class II loci. Hum. Immunol. 62:75-84. [PubMed]
Articles from Infection and Immunity are provided here courtesy of
American Society for Microbiology (ASM)