Amplified fragment length polymorphism (AFLP) analysis of closely related wild and captive tsetse fly (Glossina morsitans morsitans) populations
© Lall et al; licensee BioMed Central Ltd. 2010
Received: 10 April 2010
Accepted: 26 May 2010
Published: 26 May 2010
Tsetse flies (Diptera: Glossinidae) are vectors of trypanosomes that cause sleeping sickness in humans and nagana in livestock across sub-Saharan Africa. Tsetse control strategies rely on a detailed understanding of the epidemiology and ecology of tsetse together with genetic variation within and among populations. High-resolution nuclear genetic markers are useful tools for elucidation of the genetic basis of phenotypic traits. In this study amplified fragment length polymorphism (AFLP) markers were developed to analyze genetic variation in Glossina morsitans morsitans from laboratory and field-collected populations from Zimbabwe.
A total of seven hundred and fifty one loci from laboratory and field populations of G. m. morsitans from Zimbabwe were genotyped using AFLP with seven primer combinations. Analysis identified 335 polymorphic loci. The two populations could be distinguished by cluster and principal components analysis (PCA) analysis, indicating that AFLP markers can be used to separate genetically similar populations; at the same time differences observed between laboratory and field populations were not very great. Among the techniques investigated, the use of acetone was the most reliable method of preservation of tsetse for subsequent extraction of high molecular weight DNA. An interesting finding was that AFLP also enabled robust within-population discrimination of male and female tsetse flies due to their different X chromosome DNA complements.
AFLP represents a useful additional tool to add to the suite of techniques currently available for the genetic analysis of tsetse populations and represents a useful resource for identification of the genetic basis of important phenotypic traits.
Over the past 30 years several techniques have been used to assess the genetic variation in populations of tsetse flies, these include protein polymorphisms in house-keeping genes or allozymes [1–4], microsatellites [5–7] and mitochondrial DNA techniques [4, 6, 8–10]. The markers used in these studies have provided useful information on phenotypic and genetic polymorphism in Glossina species. In particular they have indicated a degree of genetic differentiation between geographically separated tsetse populations, which was surprising, given the mobility of the flies combined with expectations derived from population genetics theory [11–13]. Mitochondrial variation is useful for discrimination of individual flies and reveals relatively high levels of haplotype divergence between randomly chosen individuals among four species analysed, including G. morsitans. However, arthropod mitochondrial genomes are small in size (14-25 kilobases) and maternally inherited , hence data interpretation differs from that of variation in nuclear genes.
The number of tsetse loci in the nuclear genome using the techniques sampled for variation to date is relatively limited, for example in Glossina morsitans morsitans a total of 45 allozymes and five microsatellites were reported as being analysed . To provide useful genetic markers for association with phenotpyes of interest, such as vector competence, higher resolution coverage is required for Glossina species, whose estimated genome sizes range from 600 Mbp for G. morsitans to 7,000 Mbp for G. palpalis, the latter being considerably larger than the human genome . Amplified Fragment Length polymorphism (AFLP) is a fingerprinting technique that is based on selective PCR amplification of restriction fragments from a total digest of genomic DNA . It represents a powerful genotyping method that increases the utility of simple restriction enzyme digestion analysis by combining this with PCR and can typically sample 50-100 restriction enzyme fragments on a single polyacrylamide gel. Since AFLP samples polymorphism at hundreds of independent nuclear loci without any requirement for prior sequence information  the technique typically provides an in depth assessment of genome-wide variation . By contrast restriction fragment length polymorphisms (RFLPs) are restricted to sampling one locus at a time and therefore have much lower throughput than AFLPs.
The AFLP technique is a convenient and reliable tool with the capacity to discriminate closely related populations, and has been successfully applied to mosquito species and populations for genetic mapping, genotype identification, taxonomic and population genetic studies .
Population genetic studies of insect vectors such as tsetse flies requires the collection of a large number of field caught insects from remote rural locations, followed by DNA extraction and analysis. For accurate molecular analysis to be performed, it is crucial to generate DNA of good quality. It is therefore essential to identify suitable methods for maintaining the integrity of the DNA samples after collection, until extraction and analysis are performed. Tsetse flies collected for genetic analyses have in previous studies been stored in liquid nitrogen or under conditions of ultra-low temperature refrigeration [9, 19–21]. However, liquid nitrogen facilities and reliable power sources for freezer storage of materials are rarely available in areas where tsetse flies are collected and more convenient and cheaper alternative methods to preserve samples for DNA analysis are required.
The primary objective of this work was to investigate the use of AFLP as markers of genetic variation in tsetse populations, by comparing the genetic profiles of a laboratory colony, to that of a field-collected Glossina morsitans morsitans population. Multiple primer pairs were used to maximize the number of loci allowing the selection of optimal primer sets; in addition we aimed to identify a suitably inexpensive medium for storage of field-collected tsetse flies that would preserve the molecular integrity of flies so that high quality DNA could be retrieved for subsequent molecular analysis.
Electrophoresis of DNA from freshly killed flies exhibited a distinct band of high molecular weight (HMW) DNA with no low molecular weight (LMW) DNA visible. Acetone preserved flies showed a strong HMW DNA band with a limited amount of LMW DNA smearing. Flies stored in lysis buffer or ethanol-preserved flies showed a weak HMW DNA band with extensive LMW DNA smearing. Flies stored in SDS buffer or stored on FTA card matrix showed DNA profiles with LMW DNA appearing as a smear, HMW DNA band was rarely observed.
In general, electrophoresis of DNA from flies dried prior to preservation demonstrated inferior HMW DNA bands compared to freshly preserved flies. Although HMW DNA bands were detected, there was also extensive smearing in the LMW region of the gel.
DNA Yield and Purity
The preservation technique used had a significant effect on the DNA yield obtained and (GLM yield versus treatment, dried/undried: F3,63 = 9.88 p < 0.001) 260/280 nm OD ratios (GLM OD ratio versus treatment, dried/undried: F3,63 = 10.41 p < 0.001). Samples that were dried prior to preservation showed significantly reduced yields (GLM yield versus treatment, dried/undried: F1,63 = 8.68 p = 0.005) and 260/280 nm OD ratios (GLM OD ratio versus treatment, dried/undried: F1,63 = 9.8 p = 0.003) compared to freshly preserved flies. Tukey-Kramer's analysis did not demonstrate any significant difference in DNA yields or purity between acetone and ethanol treatments.
AFLP genotype analysis
Genetic variability of the tsetse populations measured by the observed number of polymorphic loci, gene diversity (heterozygosity, H) and the degree of genetic differentiation among populations (Gst).
Number of individuals
Percentage of polymorphic loci
Nei'sgene diversity h
0.21 ± 0.17
0.21 ± 0.18
0.19 ± 0.17
Cluster and PCA Analysis
Estimates of gene flow between tsetse populations based on population genetic analyses are important in the context of predicting the long-term effectiveness of tsetse control measures . However, genetic markers also have other uses, in particular as tools that can assist in determining the genetic basis underpinning important phenotypes. When captive colonies are used to analyse phenotpyes such as factors influencing vector competence [22, 23] it is important that this can be related back to the field populations.
This study demonstrates that AFLPs can be used to generate high-resolution genetic markers in natural populations of G. m. morsitans. Two distinct population groups were apparent from the cluster and PCA analysis (Figures 2 and 3). Although the separation of the two populations is not perfect, the results demonstrate that the AFLP markers can be used to separate two genetically close populations. The level of Nei's genetic diversity , h was small in both populations and the amount of genetic variation detected in the laboratory and a Zimbabwean population was similar. In addition, the GST value of 0.0386 indicates that there is little genetic differentiation between the natural Zimbabwean and the laboratory population. The results in the current study suggest that the establishment and long term maintenance of the insect colony process (> 30 years) has resulted in little effect on genetic variation as estimated by AFLPs. The fact that the flies from the laboratory colony exhibit only limited divergence from the field populations is encouraging for extrapolation of experimental results to the 'real world'. The field population did, however, show a higher number of loci and a higher percentage of polymorphic loci than the laboratory population (Table 1). AMOVA results showed that the populations are closely related as there was more variation within (91%) the populations than between (9%) them. This result, derived from variation in nuclear genes, is in agreement with that obtained for G. morsitan morsitans using mitochondrial markers . It was interesting that males and females were clearly separated using the AFLP analysis, however this can be explained by the greater DNA content of female flies where the dosage of X determines sex. Hence males are XY or XYY whereas females can be XX, XXY or XXXY . The identification of markers that can discriminate males and female flies could be valuable in the future in the identification of sex ratio distortion genes  in the tsetse genome.
Whenever possible it is preferable for DNA to be extracted from fresh tsetse material. However, when this is impractical due to location, cost or a combination of the two, the present results suggest that acetone should be used in preference to the other preservatives tested. Flies preserved in acetone gave the highest quality HMW DNA and resulted in DNA of good quality on both fresh and pre-dried material. Ethanol has been widely used for the preservation of various biological samples including insects [26–29]. In the current work both tsetse DNA yield and purity from ethanol samples were similar to acetone preserved material (Figure 1). However, ethanol preserved samples contained a low amount of HMW DNA and ethanol was inferior in the preservation of fresh flies (Figure 1). This observation is consistent with previous studies that demonstrated poor ethanol preservation in the presence of water [26, 28]. This problem was not overcome by using 100% proof ethanol and changing the ethanol after 24 h (this study).
Although the material preserved in SDS lysis buffers (either with or without proteinase K) or on a FTA card showed reasonable DNA yield and purity in all cases it was degraded LMW DNA with pronounced smearing that predominated. The LMW smearing was most extensive in the FTA samples suggesting that FTA cards are not appropriate media for storing large insects. This may be because not all parts of the fly were in contact with the matrix, allowing endonucleases activity resulting in DNA degradation.
The data presented here shows that acetone was a superior medium for preserving tsetse DNA. An additional advantage is that acetone is used as a bait component in tsetse traps and is therefore readily available to field workers collecting tsetse flies. The DNA obtained using this method could be used for PCR of specific genes, microsatellite analysis, AFLP and other molecular techniques that require high quality DNA. In addition, acetone may be an appropriate storage media for other important dipteran vectors, such as mosquitoes due to its high penetrability and dehydrating abilities. However, one of the disadvantages of using acetone is that many aircraft companies will not allow acetone to be carried in the hold.
The relative value of a range of genetic markers, specifically Random Amplification of Polymorphic DNA (RAPDs), Inter-simple-sequence repeat PCR and microsatellites as applied to the analysis of variation between strains of the silkworm (Bombyx mori) has been reviewed , although this study did not include AFLPs. The basic conclusion was that all techniques are useful and have different strengths and weaknesses in terms of factors such as resolution, ease of use and cost. As regards nuclear genetic markers in tsetse flies, allozymes sample approximately 50 loci and do reveal a degree of inter-population diversity, however they are not selectively neutral and hence may not always accurately reflect population history. Microsatellites reveal significant allelic polymorphism but are relatively few in number and are limited by the requirement for sequence data for primer design. Both have proved useful for initial analysis of inter-population differentiation in the field [11, 12]. The initial AFLP study described here has identified numerous previously unknown polymorphic loci in G. m. morsitans which as indicated above will have value in areas of tsetse research, additional to differentiation of field populations. Because these loci are essentially randomly distributed , greater in number and not necessarily selected for rapid evolution, AFLP analysis may provide a more accurate assessment of genome-wide differentiation in Glossina. In future it should prove possible to generate microsatellite markers more rapidly as expressed sequence tag and genome sequence databases  are systematically searched for variable number tandem repeat (VNTR) and single nucleotide polymorphisms (SNP). However, due to the large size of Glossina genomes  it seems likely that not all of these will have genome sequences available in the immediate future. AFLP markers which can generated over a wide dynamic range of genome sizes  should continue to be of value.
This study demonstrates the usefulness of AFLP markers in tsetse flies to assess relationships between and within tsetse populations and their potential as genetic markers for identification of the genetic basis of phenotypes. AFLP markers based on sampling hundreds of polymorphic loci are able to define differences even between closely related populations. As such, they may provide a particularly accurate technique for analysis of genetic variation and represent an additional tool for exploring the genetic diversity of tsetse populations. In the medium term application of such data this will be helpful in designing, evaluating and implementing effective tsetse control strategies to prevent trypanosomiasis.
G. m. morsitans (Westwood) originally isolated from Kariba, Zimbabwe , were obtained from long-term colonies maintained at the University of Edinburgh. This colony was set up from individuals obtained from the University of Bristol in 1996 at the University of Glasgow. In 1999 the colony from the University of Glasgow was moved to the University of Edinburgh. Since 1996 the population has fluctuated in size but the numbers have maintained between 1000 to 2500 breeding females since 2000. Glossina morsitans centralis, which was used in initial investigations to examine primer pair combinations, were obtained from the long-term colonies maintained at the International Livestock Research Institute, Nairobi, Kenya. Field collected Zimbabwean G. m. morsitans were obtained from the Rekomitjie Research Station in the Zambezi valley, near Chiuyi River, Zimbabwe (16 deg 23 min 55 s S, 29 deg 23 min 11 s E) and caught using Epsilon traps baited with acetone (500 mg/h), octenol (0.5 mg/h), 4-methylphenol (1 mg/h) and 3-n-proylphenol (0.1 mg/h). Traps were set at intervals of about 300 m and were emptied daily.
Insect material for DNA preservation
Eighty-four, colony reared G. m. morsitans were collected 20 days post-eclosion. Ten insects were used as fresh, non-preserved controls. Of the remaining 74 flies; 10 were crushed on Whatman FTA preservation matrix (Bioline Ltd., London, UK); 10 were preserved in each of the four preservation media. The preservation media used were (i) pure grade absolute acetone (99.5%); (ii) pure grade absolute ethanol (Fisher Scientific Ltd., Loughborough, UK), (iii) lysis buffer (500 mM Tris-HCl at pH 9.2, 250 mM ethylenediaminetetra-acetic acid (EDTA) and (iv) 2.5% w/v sodium dodecyl sulfate (SDS) and lysis buffer with proteinase K (50 μg/ml). Lysis buffer with proteinase K is hereafter referred to as lysis buffer P. Unless otherwise stated all chemicals and enzymes were purchased from Sigma-Aldrich, Gillingham, UK.
Field caught materials are regularly exposed to desiccation and ultraviolet radiation before collection and to simulate field conditions, 24 flies were air dried in the sun for 12 h before six were preserved in each of the four preservation media. All flies were stored individually in two ml of preservative for two months at room temperature. In the case of ethanol- and acetone-preserved samples, preservatives were replaced after the initial 24 h to ensure complete dehydration of samples.
Insect material for AFLP analysis
Fifty-nine laboratory reared G. m. morsitans and 70 field collected Zimbabwean G. m. morsitans flies were used in this study. All field-collected samples were preserved in acetone.
Flies were removed from the storage media and excess preservative removed by blotting on to absorbent paper. Whole insects were used for extraction, using a cetyltrimethylammonium bromide (CTAB) extraction method . DNA from freshly killed controls and FTA-preserved flies was extracted in the same way. Following extraction, the genomic DNA was dissolved in 50 μl of distilled water . DNA for AFLP analysis was quantified by spectrophotometry (Beckman Coulter DU 530) and diluted to a working concentration of 500 ng/μl.
DNA Quantity and Quality
Genomic DNA was subjected to spectrophotometry (Beckman Coulter DU 530) to determine yield and purity. DNA yields were calculated from concentration values while purity was determined by the 260 nm/280 nm absorbance ratio readings . Quality was accessed by running 500 ng of each sample on a 1.5% agarose gel in 1 X TBE buffer at 150 v for 30 min. The gel was stained with ethidium bromide (1 μg/ml) and bands were observed and photographed using an ultraviolet transilluminator linked to a Gel Doc 2000 BioRad system (BioRad, Hemel Hempstead, UK).
AFLP reactions were performed using the AFLP genome Plant Mapping Kit (Perkin Elmer Applied Biosystems, Warrington, UK) following the method of De Vos et al. . All adaptors and PCR primers were provided as kit components. In brief, genomic DNA was digested with EcoRI and MseI restriction enzymes. The DNA fragments were then ligated with EcoRI and MseI adaptors, generating template DNA for pre-selective PCR amplification.
The pre-selective amplification thermal cycling conditions were: an initial hold at 72°C for 2 min, followed by 20 cycles of 20 s at 94°C, 30 s at 56°C, and 2 min at 72°C with a final 30 min hold at 60°C. Following pre-selective amplification using the primer sets supplied with the kit, template for selective amplification was prepared by diluting 10 μl of each of the pre-selective amplification products with 190 μl TE buffer. Selective amplification was performed using combinations of EcoR1 and Mse1 primer pairs. Selective amplification thermal cycling conditions were: an initial denaturation at 94°C for 2 min, followed by 30 PCR cycles of 20 s at 94°C, 30 s at 66°C (10 cycles with a 1°C reduction at every cycle), 56°C (subsequent 20 cycles), and 2 min at 72°C and a final 30 min hold at 60°C.
Suitable AFLP primer combinations for G. morsitans DNA.
Mse1 primer tail
EcoR1 primer tail
AFLP alleles were detected on an ABI 3700 automatic DNA sequencer (Perkin Elmer Applied Biosystems, Beaconsfield, UK), and the AFLP allele sizes were measured using GeneMapper 3.7 software (Applied Biosystems). Binary data tables showing alleles were generated and imported into tab delimited text files. Analysis of the number, percentages of polymorphic loci and gene diversities within and across populations were calculated in Popgene . Popgene generates two estimates of heterozygosity, firstly Nei's  heterozygosity and secondly the expected heterozygosity using the algorithm of Leven  which gives the same result as Nei's  unbiased heterozygosity. Partitioning of molecular variance within and between populations was calculated by analysis of molecular variance (AMOVA) using Arlequin software .
Differences in DNA yield and purity based on the OD 260/280 nm ratio between fresh and preserved flies were analyzed using t-tests. General linear model (GLM) analysis was performed to investigate the effect of preservative and drying on DNA yield and 260/280 nm ratio. All analyses were performed with MINITAB version 14 (Minitab Ltd., Coventry UK).
Principal components analysis (PCA) and hierarchical cluster analysis were performed in R (Version 2.2.1) . Prior to the analysis, one outlier (ZIM Male 18) was excluded based on visual inspection, and the dataset was pruned to remove all non-informative alleles. Non-informative sites were defined as alleles present in all or none of the included individuals. PCA was performed on centered, non-scaled data and the hierarchical cluster analysis used Ward's minimum variance method with pairwise Manhattan distances between individuals.
We thank the UK Department for International Development (DFID) RNRRS and Research into Use Programmes for the benefit of developing countries (GKL, ETM, SCW), the Wellcome Trust (ACD, SCW) and multilateral ILRI core funds (GKL) for financial support. None of the funders had a role in the study design, data collection and analysis, decision to publish, or preparation of the manuscript. We would like to thank Steven Torr (University of Greenwich) for collecting field tsetse samples and we are grateful for the support of the International Livestock Research Institute (ILRI) tsetse unit colony, particularly the late Mr Clement Sabwa. This is ILRI publication number 200542.
- Gooding RH: Genetic polymorphism in three species of tsetse flies (Diptera: Glossinidae) in Upper Volta. Acta Trop. 1981, 38: 149-161.PubMedGoogle Scholar
- Gooding RH: Genetics of two populations of Glossina morsitans centralis (Diptera: Glossinidae) from Zambia. Acta Trop. 1989, 46: 17-22. 10.1016/0001-706X(89)90012-0.View ArticlePubMedGoogle Scholar
- Gooding RH, Mbise S, Macha P, Rolseth BM: Genetic variation in a Tanzanian population of Glossina swynnertoni (Diptera: Glossinidae). J Med Entomol. 1993, 30: 489-492.View ArticlePubMedGoogle Scholar
- Krafsur ES: Population structure of the tsetse fly Glossina pallidipes estimated by allozyme, microsatellite and mitochondrial gene diversities. Insect Mol Biol. 2002, 11: 37-45. 10.1046/j.0962-1075.2001.00307.x.PubMed CentralView ArticlePubMedGoogle Scholar
- Solano P, Duvallet G, Dumas V, Cuisance D, Cuny G: Microsatellite markers for genetic population studies in Glossina palpalis (Diptera: Glossinidae). Acta Trop. 1997, 65: 175-180. 10.1016/S0001-706X(97)00663-3.View ArticlePubMedGoogle Scholar
- Ouma JO, Cummings MA, Jones KC, Krafsur ES: Characterization of microsatellite markers in the tsetse fly, Glossina pallidipes (Diptera: Glossinidae). Mol Ecol Notes. 2003, 3: 450-453. 10.1046/j.1471-8286.2003.00480.x.PubMed CentralView ArticlePubMedGoogle Scholar
- Krafsur ES, Endsley MA: Shared microsatellite loci in Glossina morsitans sensu lato (Diptera: Glossinidae). J Med Entomol. 2006, 43: 640-642. 10.1603/0022-2585(2006)43[640:SMLIGM]2.0.CO;2.PubMed CentralView ArticlePubMedGoogle Scholar
- Krafsur ES, Griffiths N: Genetic variation at structural loci in the Glossina morsitans species group. Biochem Genet. 1997, 35: 1-11. 10.1023/A:1022252311715.View ArticlePubMedGoogle Scholar
- Krafsur ES, Wohlford DL: Breeding structure of Glossina pallidipes populations evaluated by mitochondrial variation. J Hered. 1999, 90: 635-642. 10.1093/jhered/90.6.635.View ArticlePubMedGoogle Scholar
- Marquez JG, Vreysen MJ, Robinson AS, Bado S, Krafsur ES: Mitochondrial diversity analysis of Glossina palpalis gambiensis from Mali and Senegal. Med Vet Ent. 2004, 18: 288-295. 10.1111/j.0269-283X.2004.00508.x.View ArticleGoogle Scholar
- Krafsur ES: Tsetse fly population genetics: an indirect approach to dispersal. Trends Parasitol. 2003, 19: 162-166. 10.1016/S1471-4922(03)00034-5.View ArticlePubMedGoogle Scholar
- Gooding RH, Krafsur ES: Tsetse genetics: Contributions to biology, systematics, and control of tsetse flies. Ann Rev Entomol. 2005, 50: 101-123. 10.1146/annurev.ento.50.071803.130443.View ArticleGoogle Scholar
- Krafsur ES: Tsetse flies: genetics, evolution, and role as vectors. Infect Genet Evol. 2009, 9: 124-141. 10.1016/j.meegid.2008.09.010.PubMed CentralView ArticlePubMedGoogle Scholar
- Jeyaprakash A, Hoy MA: First divergence time of spiders, scorpions, mites and ticks (sub-phylum Chelicerata) inferred from mitochondrial phylogeny. Exp Appl Acarol. 2009, 47: 1-18. 10.1007/s10493-008-9203-5.View ArticlePubMedGoogle Scholar
- Geraci NS, Johnson JS, Robinson P, Wikel SK, Hill CA: Variation in the genome size of argasid and ixodid ticks. Insect Biochem Mol Biol. 2007, 37: 399-408. 10.1016/j.ibmb.2006.12.007.View ArticlePubMedGoogle Scholar
- Vos P, Hogers R, Bleeker M, Reijans M, Lee van de T, Hornes M, Frijters A, Pot J, Peleman J, Kuiper M, Zabeau M: AFLP: a new technique for DNA fingerprinting. Nucleic Acids Res. 1995, 23: 4407-4414. 10.1093/nar/23.21.4407.PubMed CentralView ArticlePubMedGoogle Scholar
- Masiga DK, Tait A, Turner CMR: Amplified restriction fragment length polymorphism in parasite genetics. Parasitol Today. 2000, 16: 350-353. 10.1016/S0169-4758(00)01706-3.View ArticlePubMedGoogle Scholar
- Ravel S, Monteny N, Velasco Olmos D, Escalante Verdugo J, Cuny G: A preliminary study of the population genetics of Aedes aegypti (Diptera: Culicidae) from Mexico using microsatellite and AFLP markers. Acta Trop. 2001, 78: 241-250. 10.1016/S0001-706X(01)00083-3.View ArticlePubMedGoogle Scholar
- Wohlford DL, Krafsur ES, Griffiths NT, Marquez JG, Baker MD: Genetic differentiation of some Glossina morsitans morsitans populations. Med Vet Entomol. 1999, 13: 377-85. 10.1046/j.1365-2915.1999.00185.x.PubMed CentralView ArticlePubMedGoogle Scholar
- Krafsur ES, Madsen M, Wohlford DL, Mihok S, Griffiths NT: Population genetics of Glossina morsitans submorsitans (Diptera: Glossinidae). Bull Entomol Res. 2000, 90: 329-335. 10.1017/S0007485300000456.PubMed CentralView ArticlePubMedGoogle Scholar
- Krafsur ES, Endsley MA, Wohlford DL, Griffiths NT, Allsopp R: Genetic differentiation of Glossina morsitans centralis populations. Insect Mol Biol. 2001, 10: 387-95. 10.1046/j.0962-1075.2001.00277.x.PubMed CentralView ArticlePubMedGoogle Scholar
- MacLeod ET, Maudlin I, Darby AC, Welburn SC: Antioxidants promote establishment of trypanosome infections in tsetse. Parasitology. 2007, 134: 827-831. 10.1017/S0031182007002247.View ArticlePubMedGoogle Scholar
- MacLeod ET, Darby AC, Maudlin I, Welburn SC: Factors affecting trypanosome maturation in tsetse flies. PLoS One. 2007, 2: e239-10.1371/journal.pone.0000239.PubMed CentralView ArticlePubMedGoogle Scholar
- Nei M: Analysis of gene diversity in subdivided populations. Proc Natl Acad Sci USA. 1973, 70: 3321-3323. 10.1073/pnas.70.12.3321.PubMed CentralView ArticlePubMedGoogle Scholar
- Maudlin I: Chromosome polymorphism and sex determination in a wild population of tsetse. Nature. 1979, 277: 300-301. 10.1038/277300a0.View ArticlePubMedGoogle Scholar
- Post RJ, Flook PK, Millest AL: Methods for the preservation of insects for DNA studies. Biochem Syst Ecol. 1993, 21: 85-92. 10.1016/0305-1978(93)90012-G.View ArticleGoogle Scholar
- Dillon N, Austin AD, Bartowsky E: Comparison of preservation techniques for DNA extraction from hymenopterous insects. Insect Mol Biol. 1996, 5: 21-24. 10.1111/j.1365-2583.1996.tb00036.x.View ArticlePubMedGoogle Scholar
- Flournoy LE, Adams RP, Pandy RN: Interim and archival preservation of plant specimens in alcohols for DNA studies. Biotechniques. 1996, 20: 657-660.PubMedGoogle Scholar
- Quicke DLJ, Lopez-Vaamonde C, Belshaw R: Preservation of hymenopteran specimens for subsequent molecular and morphological study. Zool Scr. 1999, 28: 261-267. 10.1046/j.1463-6409.1999.00004.x.View ArticleGoogle Scholar
- Nagaraju J, Reddy KN, Nagaraja GM, Sethuraman BM: Comparison of multilocus RFLPs and PCR-based marker systems for genetic analysis of the silkworm, Bombyx mori. Heredity. 2001, 86: 588-597. 10.1046/j.1365-2540.2001.00861.x.View ArticlePubMedGoogle Scholar
- Aksoy S, Berriman M, Hall N, Hattori M, Hide W, Lehane MJ: A case for a Glossina genome project. Trends Parasitol. 2005, 21: 107-111. 10.1016/j.pt.2005.01.006.View ArticlePubMedGoogle Scholar
- Nash TA, Jordan AM, Trewern MA: The Langford colonies of tsetse flies. Trans R Soc Trop Med Hyg. 1972, 66: 308-309. 10.1016/0035-9203(72)90170-8.View ArticlePubMedGoogle Scholar
- Navajas M, Lagnel J, Gutierrez J, Boursot P: Species-wide homogeneity of nuclear ribosomal ITS2 sequences in the spider mite Tetranychus urticae contrasts with extensive mitochondrial COI polymorphism. Heredity. 1998, 80: 742-752. 10.1046/j.1365-2540.1998.00349.x.View ArticlePubMedGoogle Scholar
- Sambrook J, Fritsch EF, Maniatis T: Molecular Cloning: A Laboratory Manual. 1989, Cold Spring Harbour Laboratory Press, New YorkGoogle Scholar
- Yeh FC, Yang RC, Boyle TJB, Ye ZH, Mao JX: POPGENE, the user-friendly shareware for population genetic analysis. 1997, Edmonton, Molecular Biology and Biotechnology Centre, University of Alberta, CanadaGoogle Scholar
- Leven H: On a matching problem arising in genetics. Ann Math Statist. 1949, 20: 91-94. 10.1214/aoms/1177730093.View ArticleGoogle Scholar
- Nei M: Estimation of Average Heterozygosity and Genetic Distance from a Small Number of Individuals. Genetics. 1978, 89: 583-590.PubMed CentralPubMedGoogle Scholar
- Excoffier L, Smouse PE, Quattro JM: Analysis of molecular variance inferred from metric distances among DNA haplotypes: application to human mitochondrial DNA restriction data. Genetics. 1992, 131: 479-491.PubMed CentralPubMedGoogle Scholar
- Ross I, Gentleman R: R: A Language for Data Analysis and Graphics. J Comput Graph Stat. 1996, 5: 299-314. 10.2307/1390807.Google Scholar
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