- Research article
- Open Access
Using 454 technology for long-PCR based sequencing of the complete mitochondrial genome from single Haemonchus contortus (Nematoda)
© Jex et al; licensee BioMed Central Ltd. 2008
Received: 18 July 2007
Accepted: 11 January 2008
Published: 11 January 2008
Mitochondrial (mt) genomes represent a rich source of molecular markers for a range of applications, including population genetics, systematics, epidemiology and ecology. In the present study, we used 454 technology (or the GS20, massively parallel picolitre reactor platform) to determine the complete mt genome of Haemonchus contortus (Nematoda: Trichostrongylidae), a parasite of substantial agricultural, veterinary and economic significance. We validate this approach by comparison with mt sequences from publicly available expressed sequence tag (EST) and genomic survey sequence (GSS) data sets.
The complete mt genome of Haemonchus contortus was sequenced directly from long-PCR amplified template utilizing genomic DNA (~20–40 ng) from a single adult male using 454 technology. A single contig was assembled and compared against mt sequences mined from publicly available EST (NemBLAST) and GSS datasets. The comparison demonstrated that the 454 technology platform is reliable for the sequencing of AT-rich mt genomes from nematodes. The mt genome sequenced for Haemonchus contortus was 14,055 bp in length and was highly AT-rich (78.1%). In accordance with other chromadorean nematodes studied to date, the mt genome of H. contortus contained 36 genes (12 protein coding, 22 tRNAs, rrnL and rrnS) and was similar in structure, size and gene arrangement to those characterized previously for members of the Strongylida.
The present study demonstrates the utility of 454 technology for the rapid determination of mt genome sequences from tiny amounts of DNA and reveals a wealth of mt genomic data in current databases available for mining. This approach provides a novel platform for high-throughput sequencing of mt genomes from nematodes and other organisms.
The mitochondrion is the organelle responsible for cellular respiration and energy production in many eukaryotic organisms. In addition to its role in cellular function, the mitochondrion contains an internalised, usually circular genome (~13–20 kb in size) which is separate to, but co-operates with, the nuclear genome [1–4]. Knowledge about mt genomes and their structure provides a basis for investigating intracellular physiology and biochemistry [5, 6], and gives insights into mt disorders/diseases caused by mt gene mutations [7, 8]. Also, because the mt genome is relatively large, the genome structure is highly conserved, and many of the mt genes are highly variable, genetic markers in mt genomes are useful for taxonomic, ecological, population genetic and evolutionary studies (reviewed by [3, 4, 9]). However, for some groups of organisms, particularly invertebrates, there is very limited information on mt genomes, which most likely relates to the inaccessibility of a practical, generally applicable and cost-effective technique for mt genome sequencing. In the past, mt genome sequencing relied mainly on the purification of mtDNA from the organism under study and its subsequent cloning (with or without PCR) [10, 11], sequencing and sequence assembly to then determine the genome structure and gene order. For vertebrates and large invertebrates, where microgram or milligram amounts of mtDNA can be isolated and purified from individuals, this conventional procedure is effective. However, for small invertebrates, such as tiny parasitic worms (= helminths), the amount of mtDNA which can be purified from individuals is much too small to use this approach. Also, there can be major problems with extensive sequence variation among individuals and/or AT-richness (in some regions of the mt genome) [12, 13], preventing accurate sequence determination. An effective long PCR-based method has been established for the amplification and subsequent sequencing from individuals via primer walking . However, it has not yet been possible to directly sequence an entire mt genome sequence in a single reaction.
With the recent focus on the sequencing of complete nuclear genomes has come a substantial interest in the development of high-throughput, low cost sequencing platforms capable of much more substantial sequence outputs than has been possible with conventional sequencers. A particularly promising approach is the "massively parallel picolitre reactor platform" (or 454 technology, Life Sciences) [15–21]. The maximum total sequence length which can be determined using this method is presently ~25 Mbp , which vastly exceeds the total length of the mt genome. A recent study  demonstrated that 454 technology is more reliable than a conventional (Sanger) approach for sequencing highly AT-rich regions, suggesting that this approach could enhance long PCR-based mt genome sequencing. Moreover, the final sequence output obtained via the 454 platform can be assembled as one or more contigs from a very large number of short overlapping sequence reads, this platform may offer a more accurate output due to substantial coverage and improved bioinformatic processing following sequencing.
In the present study, we utilized a long-PCR-coupled 454 technological approach to sequence the complete mt genome from a small portion of the genomic DNA from a single adult of Haemonchus contortus (Nematoda: Strongylida). This nematode represents a blood-feeding parasite of paramount importance, as a pathogen in small ruminants (sheep and goats), causing anaemia and associated complications, leading to death in severely affected animals  and belongs to a group of nematodes (Strongylida) parasitising animals, which cause major disease problems, resulting in substantial economic losses to agricultural and livestock industries worldwide. In order to validate sequencing by this approach, we used mt data for H. contortus mined from public databases as a scaffold for mapping and assembly. Also, we characterized the mt genome of this important parasite and compared its genome structure with previously published mt genomes for other strongylid nematodes.
Results and Discussion
Molecular verification of species identity, and quality of long-PCR amplicons
A sample of total genomic DNA was isolated from a single adult male of H. contortus (McMaster strain) for the sequencing of the complete mt genome. In order to ensure the specific identity of the specimen prior to sequencing, the second internal transcribed spacer (ITS-2) of nuclear ribosomal DNA was amplified from the genomic DNA sample by the PCR and sequenced directly. The sequence obtained was identical to the ITS-2 sequence published previously for H. contortus (GenBank accession number X78803; ). Subsequently, the complete mt genome was amplified by long-PCR from the genomic DNA in two overlapping regions (~5 kb and ~10 kb, respectively) . Each amplicon appeared as one abundant band of the appropriate size on an agarose gel. Short tags (300–400 bp) were sequenced from the 10 kb and 5 kb amplicons (within the cox1 and rrnL genes, respectively) to verify their specificity and identity. Following DNA quantitation for each amplicon, the two amplicons (5 μg from each) were pooled and sequenced directly in a single reaction using 454 technology (whole genome sequencing protocol).
Validation of sequencing via 454 technology by comparison with data mined from public databases
The recently developed 454 technology platform  has been utilized for the sequencing of the complete nuclear genomes from a range of organisms [22, 25–28]. Although, prior to the present study, it had not been applied to mt genomes of nematodes, a study of marine microbes  has shown this technology (together with the Sanger method) to be particularly suited for sequencing AT-rich regions with complex secondary structures, yielding higher quality sequences and costing less overall to carry out than Sanger sequencing alone. This information indicated that 454 technology was perfectly suited to the AT-rich mt genomes of strongylid nematodes, but this required verification.
Summary of Haemonchus contortus expressed sequence tags (ESTs) mined from public databases ([30, 31]) using the full length sequence of each of the 12 protein coding genes from the mitochondrial genome obtained via 454 technology in the present study.
Gene Length (bp)
Read Length (bp)
In addition to mining EST data from online databases, GSS data (available via ) were mined for mt gene sequences using an unpublished cox1 sequence as an in silico-bait. We discovered contigs 002363 (14,442 bp) and 002480 (14,814) which were then mapped against HcMG-454 at both the nucleotide and amino acid levels (for protein coding genes), achieving complete coverage with > 99.7% similarity at the nucleotide level. Of the nucleotide differences, 6 were found within protein coding genes. Four of these single nucleotide differences between HcMG-454 and contigs 002363 and 002480 were interpreted to represent intraspecific variation in the nucleotide sequence of the mt genome of this species, as none resulted in an amino acid change. Two appeared to be sequencing errors, as they resulted in frameshifts in the inferred amino acid sequence: both were found in the cox1 gene and were base-called using alignments against available EST data (see Materials and methods section). All other nucleotide alterations (n = 34) were within non-coding regions.
Characteristics of the mt genome of Haemonchus contortus and comparative analysis with those from related nematodes
Nucleotide composition (%) for all characterised mitochondrial genomes from species of Strongylida.
AT contents (%) of the 12 protein coding genes, large and small ribosomal RNA subunits and AT-rich regions for all Strongylida for which complete mitochondrial genome data are currently available
Comparative analysis of the transcription initiation and termination codons utilized by the protein coding genes in the mitochondrial genomes of all species of Strongylida for which data are currently available.
Pairwise comparison (%) of the amino acid sequence inferred for each of the 12 protein coding mitochondrial genes from Haemonchus contortus (Hc) versus all previously described protein coding mt genes from Ancylostoma duodenale (Ad), Necator americanus (Na) and Cooperia oncophora (Co).
All circular nematode mt genomes described to date have been found to contain 22 trn genes [32, 34–37], and H. contortus is no exception (Figure 3). The trn genes for this species range from 53–61 bp, which is consistent with other nematodes [32, 34–37]. The secondary structure of the trn S genes consists of a 7–8 bp amino-acyl arm and a 5 bp anticodon stem, with a T/U residue always preceding, and a purine always following the anticodon. Twenty of the 22 trn S genes were found to have a 3–4 bp DHU arm with a 5–8 bp DHU loop and a 6–11 bp TV-replacement loop instead of a TψC arm. The two exceptions to this are the two serine (AGN and UCN) trn S genes which have a 6 bp DHU replacement loop instead of the DHU arm, and a 3–4 bp TψC arm with a 4–5 bp TψC loop instead of the TV replacement loop. These findings are consistent with the trn S genes described for all 11 chromadorean nematodes characterised to date [32, 34–37].
The rrnS and rrnL genes of H. contortus were consistent in length (702 and 915 bp, respectively) with those reported previously for most nematodes [32, 34–37], showing 77–78% and 75–76% sequence similarity, respectively, with homologous sequences from An. duodenale, N. americanus and Co. oncophora. The secondary structures for rrnS (Figure 4) and rrnL (Figure 5) were inferred by mapping against the appropriate secondary structures for N. americanus , originally based on Escherichia coli models  and predicting, either manually or through computer assisted predictions (MFOLD), changes caused by various mutations.
In accordance with the two known hookworm mt genomes , the rrnS structure consists of four relatively conserved domains (A-D, Figure 4) bound by numerous conserved helices . A 7 nt insert between positions 187–195, apparently interacts with a 7 nt tract between positions 305–311 (see Figure 4) and is predicted to result in a slight alteration of the secondary structure between conserved elements 20 and 25 , resulting in an extension of the stem between elements 20 and 22 and the formation of a 4 bp and a 7 bp stem loop between elements 23 and 25 (see Figure 4). Although the secondary structure of the rrnS of Co. oncophora was not characterised previously , the sequence did not reveal the 7 nt tract identified in H. contortus. Whether this inferred alteration in the rrnS structure in H. contortus is unique to this and/or to closely related species remains to be elucidated.
The rrnL secondary structure predicted for H. contortus is consistent with those predicted for An. duodenale and N. americanus  and consists of four major stem-loop domains (1–4) (Figure 5) which appear to be conserved [32, 34–37]. The amino-acyl trn binding sites (A) and peptidyl-transferase sites (P), first described from Escherichia coli by Noller et al.  and later recognized in nematodes , are present. Hu et al.  found that, although these "A" and "P" binding sites were present in hookworms, the exit site (E) proposed by Noller et al.  was not found in the rrnL of the hookworms or Ascaris sp., Ca. elegans, Onchocerca volvulus or Trichinella spiralis [39, 42, 43]. Also, no E site was found within the secondary structure of the rrnL of H. contortus, demonstrating consistency with previous findings and lending further support to the hypothesis that many nematode rrnL genes do not have a recognizable exit site  or, at least, not one comparable with that of E. coli . Although the secondary structure of the rrnL of Co. oncophora has not been reported previously , the sequence similarity (75–79%) among the rrnL genes of H. contortus, An. duodenale and N. americanus suggests a conserved secondary structure for these Strongylida.
Another non-coding region between cox1 and nad4 has been described from all previously characterized nematodes exhibiting gene arrangement GA2 [32, 39], namely An. duodenale, N. americanus, As. suum, S. carpocapsae and Ca. elegans. In the latter three nematodes, this region forms a stem-loop structure . However, the region does not appear to form a stem loop structure in An. duodenale nor in N. americanus , and does not appear to form a stem loop in the H. contortus mt genome reported herein. In addition, nematodes with gene arrangement GA3, presently represented by the filarial nematodes (B. malayi; accession no. AF538716), O. volvulus  and D. immitis ) from which complete mt genomes have been described, also have a gene order juxtaposed such that the cox1 gene follows the 3' end of nad4. There is no non-coding region between these two genes. This information suggests that if secondary structure in the non-coding region between cox1 and nad4 is involved in regulating replication, transcription and/or translation, it is not a universal requirement for all nematodes. Hu et al.  found a third non-coding region between the genes nad3 and nad5 (80 bp and 55 bp for An. duodenale and Ne. americanus, respectively). A similar region is present in H. contortus. In An. duodenale, this region was inferred to form a 6 bp and a 9 bp stem-loop , and it is proposed to be involved in interactions with RNA processing enzymes, as has been reported for similar stem-loop structures in humans . No such secondary structure was found for Ne. americanus , nor was it predicted here for the corresponding region in H. contortus. The degree to which such structures are involved in regulating molecular events in the mitochondria of nematodes in not yet clear and is an exciting area for future research.
454 technology as a high-throughput method for sequencing mitochondrial genomes
The present study demonstrates the utility of the 454 technology platform for the sequencing of AT-rich mt genomes combined with mapping against a scaffold of available sequences mined from public EST and/or GSS databases. This approach represents a "scaled-down" version used for sequencing complete nuclear genomes [16, 18, 20, 22, 48] and overcomes the significant limitations of sequencing AT-rich templates using conventional approaches . Presently, the equipment costs associated with this platform are likely to be prohibitive for most laboratories. Consequently, most laboratories will likely utilise commercial services if employing this method. In terms of cost, sequencing of a small number of mt genomes using this platform is probably not directly competitive with conventional Sanger sequencing via primer walking and/or cloning. However, if one considers the vast improvements, in terms of efficiency, in relation to the complete sequencing and sequence assembly of these genomes, we contend that this approach is a practical alternative.
The period from genomic DNA extraction to the final output of a complete, assembled mt genome takes ~2–3 weeks. In research applications, where a panel of conserved primers is available for primer walking, this level of output is probably achievable. However, for applications where such primers are not available (because of a lack or absence of sequence data from the organism or a related species) and must be designed de novo based on sequencing results, this present approach has major advantages. Equally, shotgun cloning-based sequencing would not be as efficient, unless a high-throughput (e.g., robotic) system were available for the rapid isolation of large numbers of clones for plasmid purification and subsequent sequencing to ensure adequate coverage of the mt genome, thus substantially increasing costs. Furthermore, by either a primer walking or shotgun cloning approach, a significant amount of bioinformatic processing is required for contig assembly following sequencing, which is not required using the 454 platform because contig assembly is automated. Economically, if 454 technology is applied as a high-throughput system in which multiple mt genomes are sequenced simultaneously, the direct costs per such genome (~USD 1,250) becomes directly comparable with, if not less expensive than other approaches. The benefits in terms of efficiency presented by this technology are considered substantial.
In addition to cost and efficiency benefits, the 454 sequencing method may provide greater reliability in the sequence output (estimated sequencing error in the present study was 2 errors in 14,055 bp of sequence) which will likely improve as newer versions (e.g., the GS-FLX system) of the sequencing platform and assembly software are made available. Given the cost and laborious nature of primer walking and/or conventional cloning-based methods, most mt genomes presently available have been assembled as a single contig following uni- or bi-directional sequencing, resulting in a one- to two-fold coverage of the genome (forward and reverse strands). The sequencing of large numbers of overlapping sequences generated from a template using the 454 technology offers a substantial increase in coverage. In the present study, the complete mt genome was assembled from ~6,000 overlapping sequences, each read being ~100 bp . This translates into a total sequence output from one reaction of ~600,000 bp, resulting in substantial "coverage" of the mitochondrial genome, which would be impractical, too laborious and costly to achieve using conventional sequencing approaches.
Previously, it has been suggested that the 454 technology may be less reliable for sequencing homopolymeric and repetitive elements [18, 22], which have been detected previously in the mt genomes of nematodes, particularly in the AT-rich region . In the mt genome of H. contortus determined, 66 such regions (of 7–9 As or Ts) were identified, but there was no evidence (based on comparison with EST and GSS datasets) of any problems herein with sequencing through such elements. In the present study, the discovery of a complete mt genome sequence for H. contortus in a GSS database allowed the direct evaluation of the 454 sequencing output, and did not reveal any sequencing errors. As homopolymeric and repetitive elements can occur in the AT-rich region and elsewhere, it may be warranted, for organisms for which no prior sequence data are available, to undertake conventional Sanger sequencing to independently verify the accuracy of such sequence elements determined by 454 technology.
The present study demonstrates clearly the utility and practicality of 454 technology for the sequencing of mt genomes. The high-throughput capacity of this approach provides unique prospects for large-scale mt sequencing projects as a foundation for population genetic, evolutionary and ecological studies . The present investigation also discovered substantial amounts of mt data present in EST and GSS data sets for H. contortus, suggesting that databases available for other species will provide a useful resource for the mining of data to assist in the annotation, assembly and analyses of mt genome sequence data.
The sequence (HcMG-454) reported in this paper is available in the GenBank database under accession number EU346694.
Production of Haemonchus contortus, isolation of genomic DNA and verification of specific identity by molecular means
Adults of H. contortus (McMaster strain) were produced in a helminth-free sheep . Adult worms were isolated from the abomasum (= stomach) and washed extensively in physiological saline (25°C). Using a dissecting microscope (5× magnification), the sex of individual worms was verified microscopically, and male and female worms separated. Individual worms were transferred to sterile, screw-top cryogenic tubes (Nunc) and frozen (-70°C) in a minimal amount of buffer. After thawing, total genomic DNA was isolated from an individual male of H. contortus using a standard sodium dodecyl-sulphate/proteinase K treatment , followed by purification over a mini-column (Wizard, Promega). The specific identity of the specimen was verified by PCR-based amplification of the second internal transcribed spacer (ITS-2) of nuclear ribosomal DNA using an established method, followed by mini-column purification of the amplicon and subsequent automated sequencing (BigDye chemistry v3.1) ; the ITS-2 sequence determined was identical to that with GenBank accession no. X78803 .
Long-PCR amplification of two mt genome regions
The complete mt genome was amplified from ~10% (20–40 ng) of the genomic DNA from the individual specimen by long-PCR (BD Advantage 2; BD Biosciences) as two overlapping amplicons (large and small), using the protocol described by Hu et al.  with minor modifications. The large (~10 kb) amplicon was produced using the primers MH43F (forward: 5'-TTCTTATGAGATTGCTTTTTCT-3') and MH40R (reverse: 5'-GAATTAAACTAATATCACGT-3'). Briefly, the PCR (50 μl) was conducted using 10 pmol of each of the two oligonucleotide primers, 100 μM of each dNTP, 3 mM MgCl2 and 1 U of BD Advantage 2 Taq polymerase (BD Biosciences) using an ABI 2720 thermal cycler (ABI), employing the following cycling protocol: one cycle at 94°C for 2 min (initial denaturation), followed by 35 cycles of 94°C for 30 s (denaturation), 50°C for 30 s (annealing) and 65°C for 10 min (extension), followed by a final extension at 65°C for 10 min (utilizing the appropriate positive and negative controls). The small (~5 kb) amplicon was generated using the primer set MH39F (forward: 5'-TAAATGGCAGTCTTAGCGTGA-3') and MH38R (reverse: 5'-TAAATGGCAGTCTTAGCGTGA-3') under the same conditions, with the exception that the extension temperature was reduced to 60°C . The specificity of the two primer sets had been validated previously . Following the PCR, each amplicon was subjected to electrophoresis in 1% agarose, using a 1 kb DNA Ladder (Promega) to estimate size. Amplicons were then purified over a mini-column (Wizard, Promega) and quantified spectrophotometrically using a NanoDrop ND-1000 UV-VIS spectrophotometer v.3.2.1 (NanoDrop Technologies). The specificity of the PCR conditions and amplicons was verified by partial, automated Sanger sequencing (employing BigDye Chemistry v3.1), using primers COIF (5'-TTTTTTGGGCATCCTGAGGTTTAT-3') and MH28R (5'-CTAACTACATAATAAGTATCATG-3') (large fragment) and MH37F (5'-GGAGTAAAGTTGTATTTAAAC-3') and MH40R (5'-GAATTAAACTAATATCACGT-3') (small fragment) [3, 35].
Automated sequencing using 454 technology
The two amplicons (~5 kb and 10 kb; 5 μg of each) spanning the mt genome of H. contortus were pooled and subsequently sequenced using the Genome Sequencer 20 (GS 20; Roche) according to the protocol provided . The mt genome sequence (designated HcMG-454; GenBank accession no. EU346694) was assembled automatically and compared against EST and GSS sequences for H. contortus available from public databases [30, 31]. HcMG-454 was scanned for open reading frames (ORFs) using ORFinder , employing the "Invertebrate Mitochondrial" option. Protein coding genes were identified by BLASTx analysis of the inferred amino acid sequences, and the initiation and termination codons identified by alignment at the nucleotide (ClustalX) and amino acid (Clustal W) levels against the mostly closely related nematode species for which the mt genome has been characterized. The positions and secondary structures of all transfer RNA (trn) genes were identified or determined using tRNAscan SE 1.21  using the "Nematode Mito" source option and the "Invertebrate Mito" tRNA isotype prediction option. The rrnL and rrnS genes and AT-rich control region were identified by BLASTn analysis and comparisons with respective sequences within the mt genomes of An. duodenale, Ne. americanus, Co. oncophora and Ce. elegans (see GenBank accession numbers AJ417718, AJ417719, AY265417 and X54252, respectively). The secondary structures for the rrnL and rrnS were predicted by sequence alignment against rrnL and rrnS from Ne. americanus  with secondary structures for variable regions determined using MFOLD . The secondary structure of the AT-rich region was also determined using MFOLD. Following genome annotation, each protein-coding gene was conceptually translated using Translation Tool (v.3.1)  using the Invertebrate Mitochondrial Code" option. Amino acid sequences were aligned with those inferred from previously characterised mt genomes for species of Strongylida (i.e., An. duodenale, Ne. americanus and Co. oncophora) and C. elegans using Clustal W , adjusted manually and verified using BioEdit v.7.0.3 .
This project was supported by the Australian Research Council (LX0775848). Thanks to Ian Smith and Noel Cogan for support.
- Le TH, Blair D, McManus DP: Mitochondrial genomes of parasitic flatworms. Trends Parasitol. 2002, 18: 206-213. 10.1016/S1471-4922(02)02252-3.View ArticleGoogle Scholar
- Boore JL: Animal mitochondrial genomes. Nucleic Acids Res. 1999, 27: 1767-1780. 10.1093/nar/27.8.1767.PubMed CentralView ArticleGoogle Scholar
- Hu M, Chilton NB, Gasser RB: The mitochondrial genomics of parasitic nematodes of socio-economic importance: recent progress, and implications for population genetics and systematics. Adv Parasitol. 2004, 56: 133-212.View ArticleGoogle Scholar
- Hu M, Gasser RB: Mitochondrial genomes of parasitic nematodes--progress and perspectives. Trends Parasitol. 2006, 22: 78-84. 10.1016/j.pt.2005.12.003.View ArticleGoogle Scholar
- Wang XO: The expanding role of mitochondria in apoptosis. Genes Dev. 2001, 15: 2922-2933.Google Scholar
- Desagher S, Martinou JC: Mitochondria as the central control point of apoptosis. Trends Cell Biol. 2000, 10:Google Scholar
- Nardin RA, Johns DR: Mitochondrial dysfunction and neuromuscular disease. Muscle Nerve. 2001, 24: 170-191. 10.1002/1097-4598(200102)24:2<170::AID-MUS30>3.0.CO;2-0.View ArticleGoogle Scholar
- Larsson NG, Clayton DA: Molecular genetic aspects of human mitochondrial disorders. Annu Rev Genet. 1995, 29: 151-178. 10.1146/annurev.ge.29.120195.001055.View ArticleGoogle Scholar
- Le TH, Blair D, McManus DP: Mitochondrial genomes of human helminths and their use as markers in population genetics and phylogeny. Acta Trop. 2000, 77: 243-256. 10.1016/S0001-706X(00)00157-1.View ArticleGoogle Scholar
- Burger G, Lavrov DV, Forget L, Lang BF: Sequencing complete mitochondrial and plastid genomes. Nat Protoc. 2007, 2 (3): 603-614. 10.1038/nprot.2007.59.View ArticleGoogle Scholar
- Lang BF, Burger G: Purification of mitochondrial and plastid DNA. Nature Protocols. 2007, 2: 652-660. 10.1038/nprot.2007.58.View ArticleGoogle Scholar
- Anderson TC, Blouin MS, Beech RN: Population biology of parasitic nematodes: applications of genetic markers. Adv Parasitol. 1998, 41: 219-283.View ArticleGoogle Scholar
- Blouin MS, Yowell CA, Courtney CH, Dame JB: Substitution bias, rapid saturation, and the use of mtDNA for nematode systematics. Mol Biol Evol. 1998, 15: 1719-1727.View ArticleGoogle Scholar
- Hu M, Chilton NB, Gasser RB: Long PCR-based amplification of the entire mitochondrial genome from single parasitic nematodes. Mol Cell Probes. 2002, 16: 261-267. 10.1006/mcpr.2002.0422.View ArticleGoogle Scholar
- Cheung F, Haas BJ, Goldberg SM, May GD, Xiao Y, Town CD: Sequencing Medicago truncatula expressed sequenced tags using 454 Life Sciences technology. BMC Genomics. 2006, 7: 272-10.1186/1471-2164-7-272.PubMed CentralView ArticleGoogle Scholar
- Wicker T, Schlagenhauf E, Graner A, Close TJ, Keller B, Stein N: 454 sequencing put to the test using the complex genome of barley. BMC Genomics. 2006, 7: 275-10.1186/1471-2164-7-275.PubMed CentralView ArticleGoogle Scholar
- Edwards RA, Rodriguez-Brito B, Wegley L, Haynes M, Breitbart M, Peterson DM, Saar MO, Alexander S, Alexander EC, Rohwer F: Using pyrosequencing to shed light on deep mine microbial ecology. BMC Genomics. 2006, 7: 57-10.1186/1471-2164-7-57.PubMed CentralView ArticleGoogle Scholar
- Margulies M, Egholm M, Altman WE, Attiya S, Bader JS, Bemben LA, Berka J, Braverman MS, Chen YJ, Chen Z, Dewell SB, Du L, Fierro JM, Gomes XV, Godwin BC, He W, Helgesen S, Ho CH, Irzyk GP, Jando SC, Alenquer ML, Jarvie TP, Jirage KB, Kim JB, Knight JR, Lanza JR, Leamon JH, Lefkowitz SM, Lei M, Li J, Lohman KL, Lu H, Makhijani VB, McDade KE, McKenna MP, Myers EW, Nickerson E, Nobile JR, Plant R, Puc BP, Ronan MT, Roth GT, Sarkis GJ, Simons JF, Simpson JW, Srinivasan M, Tartaro KR, Tomasz A, Vogt KA, Volkmer GA, Wang SH, Wang Y, Weiner MP, Yu P, Begley RF, Rothberg JM: Genome sequencing in microfabricated high-density picolitre reactors. Nature. 2005, 437: 376-380.PubMed CentralGoogle Scholar
- Green RE, Krause J, Ptak SE, Briggs AW, Ronan MT, Simons JF, Du L, Egholm M, Rothberg JM, Paunovic M, Paabo S: Analysis of one million base pairs of Neanderthal DNA. Nature. 2006, 444: 330-336. 10.1038/nature05336.View ArticleGoogle Scholar
- Noonan JP, Coop G, Kudaravalli S, Smith D, Krause J, Alessi J, Chen F, Platt D, Paabo S, Pritchard JK, Rubin EM: Sequencing and analysis of Neanderthal genomic DNA. Science. 2006, 314: 1113-1118. 10.1126/science.1131412.PubMed CentralView ArticleGoogle Scholar
- Poinar HN, Schwarz C, Qi J, Shapiro B, Macphee RD, Buigues B, Tikhonov A, Huson DH, Tomsho LP, Auch A, Rampp M, Miller W, Schuster SC: Metagenomics to paleogenomics: large-scale sequencing of mammoth DNA. Science. 2006, 311: 392-394. 10.1126/science.1123360.View ArticleGoogle Scholar
- Goldberg SM, Johnson J, Busam D, Feldblyum T, Ferriera S, Friedman R, Halpern A, Khouri H, Kravitz SA, Lauro FM, Li K, Rogers YH, Strausberg R, Sutton G, Tallon L, Thomas T, Venter E, Frazier M, Venter JC: A Sanger/pyrosequencing hybrid approach for the generation of high-quality draft assemblies of marine microbial genomes. Proc Natl Acad Sci U S A. 2006, 103: 11240-11245. 10.1073/pnas.0604351103.PubMed CentralView ArticleGoogle Scholar
- Newton SE, Munn EA: The development of vaccines against gastrointestinal nematode parasites, particularly Haemonchus contortus. Parasitol Today. 1999, 15: 116-122. 10.1016/S0169-4758(99)01399-X.View ArticleGoogle Scholar
- Stevenson LA, Chilton NB, Gasser RB: Differentiation of Haemonchus placei from H. contortus (Nematoda: Trichostrongylidae) by the ribosomal DNA second internal transcribed spacer. Int J Parasitol. 1995, 25: 483-488. 10.1016/0020-7519(94)00156-I.View ArticleGoogle Scholar
- Pinard R, de Winter A, Sarkis GJ, Gerstein MB, Tartaro KR, Plant RN, Egholm M, Rothberg JM, Leamon JH: Assessment of whole genome amplification-induced bias through high-throughput, massively parallel whole genome sequencing. BMC Genomics. 2006, 7: 216-10.1186/1471-2164-7-216.PubMed CentralView ArticleGoogle Scholar
- Moore MJ, Dhingra A, Soltis PS, Shaw R, Farmerie WG, Folta KM, Soltis DE: Rapid and accurate pyrosequencing of angiosperm plastid genomes. BMC Plant Biol. 2006, 6: 17-10.1186/1471-2229-6-17.PubMed CentralView ArticleGoogle Scholar
- Leininger S, Urich T, Schloter M, Schwark L, Qi J, Nicol GW, Prosser JI, Schuster SC, Schleper C: Archaea predominate among ammonia-oxidizing prokaryotes in soils. Nature. 2006, 442: 806-809. 10.1038/nature04983.View ArticleGoogle Scholar
- Oh JD, Kling-Backhed H, Giannakis M, Xu J, Fulton RS, Fulton LA, Cordum HS, Wang C, Elliott G, Edwards J, Mardis ER, Engstrand LG, Gordon JI: The complete genome sequence of a chronic atrophic gastritis Helicobacter pylori strain: evolution during disease progression. Proc Natl Acad Sci U S A. 2006, 103: 9999-10004. 10.1073/pnas.0603784103.PubMed CentralView ArticleGoogle Scholar
- Parkinson J, Mitreva M, Whitton C, Thomson M, Daub J, Martin J, Schmid R, Hall N, Barrell B, Waterston RH, McCarter JP, Blaxter ML: A transcriptomic analysis of the phylum Nematoda. Nat Genet. 2004, 36: 1259-1267. 10.1038/ng1472.View ArticleGoogle Scholar
- sanger: The Wellcome Trust Sanger Institute. [http://www.sanger.ac.uk/Projects/H_contortus]
- nembase: NemBase, Washington University. [http://www.nematodes.net]
- Hu M, Chilton NB, Gasser RB: The mitochondrial genomes of the human hookworms, Ancylostoma duodenale and Necator americanus (Nematoda: Secernentea). Int J Parasitol. 2002, 32: 145-158. 10.1016/S0020-7519(01)00316-2.View ArticleGoogle Scholar
- Van der Veer M, de Vries E: A single nucleotide polymorphism map of the mitochondrial genome of the parasitic nematode Cooperia oncophora. Parasitology. 2004, 128: 421-431. 10.1017/S0031182003004633.View ArticleGoogle Scholar
- He Y, Jones J, Armstrong M, Lamberti F, Moens M: The mitochondrial genome of Xiphinema americanum sensu stricto (Nematoda: Enoplea): considerable economization in the length and structural features of encoded genes. J Mol Evol. 2005, 61: 819-833. 10.1007/s00239-005-0102-7.View ArticleGoogle Scholar
- Hu M, Chilton NB, Gasser RB: The mitochondrial genome of Strongyloides stercoralis (Nematoda) - idiosyncratic gene order and evolutionary implications. Int J Parasitol. 2003, 33: 1393-1408. 10.1016/S0020-7519(03)00130-9.View ArticleGoogle Scholar
- Hu M, Gasser RB, Abs El-Osta YG, Chilton NB: Structure and organization of the mitochondrial genome of the canine heartworm, Dirofilaria immitis. Parasitology. 2003, 127: 37-51. 10.1017/S0031182003003275.View ArticleGoogle Scholar
- Keddie EM, Higazi T, Boakye D, Merriweather A, Wooten MC, Unnasch TR: Onchocerca volvulus: limited heterogeneity in the nuclear and mitochondrial genomes. Exp Parasitol. 1999, 93: 198-206. 10.1006/expr.1999.4450.View ArticleGoogle Scholar
- Kim KH, Eom KS, Park JK: The complete mitochondrial genome of Anisakis simplex (Ascaridida: Nematoda) and phylogenetic implications. Int J Parasitol. 2006, 36: 319-328. 10.1016/j.ijpara.2005.10.004.View ArticleGoogle Scholar
- Montiel R, Lucena MA, Medeiros J, Simoes N: The complete mitochondrial genome of the entomopathogenic nematode Steinernema carpocapsae: insights into nematode mitochondrial DNA evolution and phylogeny. J Mol Evol. 2006, 62: 211-225. 10.1007/s00239-005-0072-9.View ArticleGoogle Scholar
- Okimoto R, Macfarlane JL, Clary DO, Wolstenholme DR: The mitochondrial genomes of two nematodes, Caenorhabditis elegans and Ascaris suum. Genetics. 1992, 130: 471-498.PubMed CentralGoogle Scholar
- Dams E, Hendriks L, Van de Peer Y, Neefs JM, Smits G, Vandenbempt I, De Wachter R: Compilation of small ribosomal subunit RNA sequences. Nucleic Acids Res. 1988, 16 Suppl: r87-r173.View ArticleGoogle Scholar
- Noller HF, Asire M, Barta A, Douthwaite S, Goldstein T, Gutell RR, Moazed D, Normanly J, Prince JB, Stern S, Triman K, Turner S, Van Stolk B, Wheaton V, Weiser B, Woese CR: Studies on the structure and function of ribosomal RNA. Structure, Function and Genetics of Ribosomes. Edited by: Hardesty BKG. 1986, New York, Springer-Verlag, 143-163.View ArticleGoogle Scholar
- Keddie EM, Higazi T, Unnasch TR: The mitochondrial genome of Onchocerca volvulus: sequence, structure and phylogenetic analysis. Mol Biochem Parasitol. 1998, 95: 111-127. 10.1016/S0166-6851(98)00102-9.View ArticleGoogle Scholar
- Lavrov DV, Brown WM: Trichinella spiralis mtDNA: a nematode mitochondrial genome that encodes a putative ATP8 and normally structured tRNAS and has a gene arrangement relatable to those of coelomate metazoans. Genetics. 2001, 157: 621-637.PubMed CentralGoogle Scholar
- Zhang DX, Hewitt DM: Insect mitochondrial control region: a review of its structure, evolution and usefulness in evolutionary studies. Biochem Syst Evol. 1997, 25: 99-120. 10.1016/S0305-1978(96)00042-7.View ArticleGoogle Scholar
- Lewis DL, Farr CL, Farquhar AL, Kaguni LS: Sequence, organization, and evolution of the A+T region of Drosophila melanogaster mitochondrial DNA. Mol Biol Evol. 1994, 11 (3): 523-538.Google Scholar
- Anderson S, Bankier AT, Barrell BG, de Bruijn MH, Coulson AR, Drouin J, Eperon IC, Nierlich DP, Roe BA, Sanger F, Schreier PH, Smith AJ, Staden R, Young IG: Sequence and organization of the human mitochondrial genome. Nature. 1981, 290 (5806): 457-465. 10.1038/290457a0.View ArticleGoogle Scholar
- Ojala D, Montaya J, Attardi G: tRNA punctuation model of RNA processing in human mitochondria. Nature. 1981, 290: 470-474. 10.1038/290470a0.View ArticleGoogle Scholar
- Angly FE, Felts B, Breitbart M, Salamon P, Edwards RA, Carlson C, Chan AM, Haynes M, Kelley S, Liu H, Mahaffy JM, Mueller JE, Nulton J, Olson R, Parsons R, Rayhawk S, Suttle CA, Rohwer F: The marine viromes of four oceanic regions. PLoS Biol. 2006, 4: e368-10.1371/journal.pbio.0040368.PubMed CentralView ArticleGoogle Scholar
- Nikolaou S, Hartman D, Presidente PJ, Newton SE, Gasser RB: HcSTK, a Caenorhabditis elegans PAR-1 homologue from the parasitic nematode, Haemonchus contortus. Int J Parasitol. 2002, 32: 749-758. 10.1016/S0020-7519(02)00008-5.View ArticleGoogle Scholar
- Gasser RB, Chilton NB, Hoste H, Beveridge I: Rapid sequencing of rDNA from single worms and eggs of parasitic helminths. Nucleic Acids Res. 1993, 21: 2525-2526. 10.1093/nar/21.10.2525.PubMed CentralView ArticleGoogle Scholar
- Schindler AR, de Gruijter JM, Polderman AM, Gasser RB: Definition of genetic markers in nuclear ribosomal DNA for a neglected parasite of primates, Ternidens deminutus (Nematoda: Strongylida)--diagnostic and epidemiological implications. Parasitology. 2005, 131: 539-546. 10.1017/S0031182005007936.View ArticleGoogle Scholar
- orfinder: ORFinder. [http://www.ncbi.nlm.nih.gov]
- trnascan: tRNAscan SE 1.21. [http://lowelab.ucsc.edu/tRNAscan-SE/]
- Zuker M, Mathews DH, Turner DH: Algorithms and Thermodynamics for RNA Secondary Structure Prediction: A Practical Guide in RNA Biochemistry and Biotechnology. NATO ASI Series. Edited by: Barciszewski J and Clark BFC. 1999, , Kluwer Academic PublishersGoogle Scholar
- translation: Translation Tool (v.3.1). [http://www.bioinformatics.vg/bioinformatics_tools/tranlatetool.shtml]
- Thompson JD, Gibson TJ, Plewniak F, Jeanmougin F, Higgins DG: The Clustal X windows interface: flexible strategies for multiple sequence alignment aided by quality analysis tools. Nucleic Acids Research. 1997, 24: 4876-4882. 10.1093/nar/25.24.4876.View ArticleGoogle Scholar
- bioedit: BioEdit v.7.0.3. [http://www.mbio.ncsu.edu/BioEdit/bioedit.html]
This article is published under license to BioMed Central Ltd. This is an Open Access article distributed under the terms of the Creative Commons Attribution License (http://creativecommons.org/licenses/by/2.0), which permits unrestricted use, distribution, and reproduction in any medium, provided the original work is properly cited.