Losing helena: The extinction of a drosophila line-like element
© Rebollo et al; licensee BioMed Central Ltd. 2008
Received: 31 October 2007
Accepted: 31 March 2008
Published: 31 March 2008
Transposable elements (TEs) are major players in evolution. We know that they play an essential role in genome size determination, but we still have an incomplete understanding of the processes involved in their amplification and elimination from genomes and populations. Taking advantage of differences in the amount and distribution of the Long Interspersed Nuclear Element (LINE), helena in Drosophila melanogaster and D. simulans, we analyzed the DNA sequences of copies of this element in samples of various natural populations of these two species.
In situ hybridization experiments revealed that helena is absent from the chromosome arms of D. melanogaster, while it is present in the chromosome arms of D. simulans, which is an unusual feature for a TE in these species. Molecular analyses showed that the helena sequences detected in D. melanogaster were all deleted copies, which diverged from the canonical element. Natural populations of D. simulans have several copies, a few of them full-length, but most of them internally deleted.
Overall, our data suggest that a mechanism that induces internal deletions in the helena sequences is active in the D. simulans genome.
Genome evolution occurs by several processes, including global genome duplications, segmental duplications and the amplification/deletion of repetitive sequences. Among the repeated sequences, transposable elements (TEs), which constitute a high proportion in many genomes, play an important role in genome evolution . The transposition rates of these TEs depend on the amount and type of the TEs present in the genome; they are not constant over time, but are subject to amplification bursts in certain species and populations . As a result, genomes contain widely differing amounts of TEs that are not directly correlated to their activity levels. For instance, the human genome is composed of at least 50% of TEs, but only very few are active, and they are responsible for less than 1% of mutations . In contrast, in Drosophila melanogaster, only 18% of the genome is composed of TEs, but a high proportion of mutations (more than 50%) is attributable to their transposition .
A TE life cycle can be viewed as successive waves of transposition/loss: invasion of the host genome by TEs being followed by their progressive elimination [5, 6]. For example, the LINE-1 (L1) element has colonized the entire human genome by successful waves of transposition [2, 7], and today it is the most abundant TE family in this genome. However, in humans, most of the elements have been inactivated either by structural changes or by epigenetic control, such as DNA methylation . In D. melanogaster, the I factor has recently reinvaded this genome after being lost from the chromosome arms . TE elimination from genomes is therefore a commonly observed phenomenon, although no real-time observation of a TE extinction has ever been reported. As TEs have a considerable influence on remodeling the genome structure , we need to understand the dynamics of changes in their copy numbers. One way to investigate these dynamics is to analyze closely related species with differing TE amounts, such as D. simulans and D. melanogaster. These species diverged 2 to 3 million years ago  and have differing proportions of TEs: D. melanogaster contains more than 18% of TEs, whereas D. simulans contains only 5% .
D. simulans has fewer copies of most TEs , but there are a few exceptions. The DNA-transposon hobo is more abundant in D. simulans, the retrovirus-like gypsy and ZAM elements have the same low number of copies in both species, and the LINE-like element helena is present in the D. simulans genome (10 insertion sites as determined by in situ hybridization), but has not been detected in the chromosome arms of D. melanogaster [11, 12]. The striking distribution of helena in natural populations of these two species, and the fact that degenerated copies are found in the sequenced D. melanogaster genome, make this LINE-like element an ideal model system to study the real time TE life cycle.
Petrov and colleagues  proposed that deletions are common events in Drosophila, and based this suggestion on the analysis of partial helena sequences from different Drosophila species. However, it is difficult to extrapolate this to other TEs, if we take into account the fact that helena is one of the few degenerate TEs in the D. melanogaster sequenced genome . Comparing closely related species with differing TE amounts, could be used to test the importance of this deletion process in regulating TE genome invasions.
We analyzed the structure and activity of helena using the sequenced genomes and of 41 natural populations of D. melanogaster and D. simulans. We show that the elimination of helena from its host genomes is a very quick process, and that it is mediated by massive internal deletions in the element . We conclude that the process of elimination of helena is far advanced in D. melanogaster. but is still in progress in D. simulans.
In silico identification of a complete copy of helena in the D. simulans genome
The copies of helena in the sequenced genomes of D. melanogaster and D. simulans
Using the complete sequence of helena as a query, we found 62 helena sequences in the D. simulans genome (see Additional File 1 for details). Twenty-eight of these copies were located on the chromosome arms, and the remaining 34 were in the U part of the genome, that may correspond to heterochromatin. The copies ranged in size from 107 bp to 5098 bp. However, it is difficult to determine the exact size of some copies due to the presence of numerous undetermined bases. Two copies (chr2R_13305831 and chrX_16602314) were longer than the reference sequence due to insertions. In some other cases, we may be looking at fragments of the same copy; however, the distances that separate them are too large to allow us to find out with certainty whether they come from the same copy. The estimated number of 62 copies in D. simulans may therefore be an overestimation. The average percentage identity is 96.1% for all copies, with an average of 97.4% for the copies in the euchromatin, and of 94.9% for the copies in the U part.
In the sequenced genome of D. melanogaster, we found 26 copies of helena (see Additional File 2 for details), which ranged in size from 91 bp to 4805 bp. The average percentage identity was 80.4% for all copies, with an average of 78.7% for the copies in the chromosome arms, and of 83.7% for the copies located in the U part. Most of the copies in this genome have therefore been degraded, with numerous internal deletions or insertions. All copies are truncated on the 5' side, and are DOA (Dead on arrival) copies, apart from the 3L_23487977 copy, although even this displays some internal deletions.
Chromatin localization of helena copies in natural populations
We used in situ hybridization to estimate the number of helena insertion sites located on the arms (euchromatin) of the polytene chromosomes from salivary glands of both D. melanogaster and D. simulans. Both species had centromeric staining, but only D. simulans from natural populations presented euchromatic bands (mean copy number 10.7 ± 2.2) with no fixed sites (see Additional File 3 for details on insertion sites per population). With this experiment we did not detect any insertions of helena in the chromosome arms, which could be explained by the short size of the elements and the divergence to the probe used.
Three sets of primers were used to amplify the whole ORF1 and two fragments of the ORF2. No bands corresponding to the ORF1 were observed in any of the D. melanogaster natural populations in agreement with the absence of this ORF in the sequenced genome. There was a high level of size polymorphism for the D. melanogaster ORF2, corresponding to the different internal deletions already analyzed by Petrov et al. [13, 23]. In contrast, D. simulans displayed low size polymorphism for helena ORF1 and ORF2. Indeed, only one population out of twenty had two sets of ORF1 (Papeete). All D. simulans populations had two to three sets of ORF2.
Analysis of helena copies in D. simulans populations
The percentage identity between the reference copy and ORF1 ranges between 96% and 99%, meaning that these copies have not diverged much. No relationship was detected between the size and location of the deletions, and the percentage identity. For the ORF2, we found copies with a percentage identity of more than 93% that reached 100% for some copies. A common 401-bp deletion was found in copies with 93% identity with the complete helena copy, but no correlation was observed with the percentage identity for the other deletions or insertions. Based on the age estimation of each copy, we found that most of the oldest ORF2 fragments had the 401-bp deletion. Several young copies of both ORF1 and ORF2 displayed major internal deletions, showing that the mechanism leading to these deletions is much more powerful than copy divergence in inactivating them.
Transcript analysis in D. simulans
To test the transcriptional potential of helena in D. simulans, we performed northern blot and RT-PCR in various populations (see Materials and Methods). Since the sequenced genome was obtained from strains from North America, we added three populations from this continent (San Antonio, SW3-S2 and San Diego). No transcripts were found by Northern blot in any of the populations. However, the RT-PCR method detected transcripts of both ORF1 and ORF2 in the Valence population, an extremely low signal for ORF1 and ORF2 in three of the American populations, and ORF2 transcripts in the Amieu population. None of the other populations had any transcript for helena, implying that this element is extinct in these populations. Since the Northern blot technique is less sensitive than RT-PCR, these findings suggest that helena is transcribed at extremely low levels in the populations in which some transcripts were detected by RT-PCR.
Our in silico and experimental analyses of the D. melanogaster genome show that helena copies are mostly DOA, devoid of ORF1, and therefore unable to transpose autonomously. All these features have been associated with elements that are in the process of inactivation . The scenario for the helena copies in D. simulans is quite different. Analysis of the sequenced genome of this species allowed us to identify a full-length copy of helena with the structures required for an active element: two intact ORFs, a poly-A tail, and regulatory regions. The high level of insertion polymorphism detected in the natural populations suggests that helena is an active element or has been active recently. However, sequence analysis of the two ORFs of helena in the natural populations revealed two main points: first, both ORFs are intact in only very few populations; second, even though the sequences of helena are very similar at the nucleotide level, their deletion features differ.
The first point was strengthened by the almost total absence of helena transcripts in all natural populations of D. simulans, which means that very few copies were involved in transcription. Because a single master copy is enough to maintain TE transposition , the putative activity of helena in this species could reside in the full-length copy probably present in some populations such as Valence, where we did observe transcripts. Hence, we would expect sequences that are still similar at nucleotide level to differ only in the 5' end truncation size, as usually observed for LINE-like elements. However, as mentioned in the second point, we actually observed many other kinds of internal deletions that occurred throughout the length of the element. Intriguingly this deletion-promoting process appears to be quite powerful in inactivating the elements, and could be even more powerful than other mutation processes such as point mutations. This means that a real-time loss of helena is ongoing in all D. simulans populations.
The nature of the mechanisms leading to internally deleted copies is still unknown. In humans, LINE elements can be spliced , a process that creates internal deletions. We used bioinformatic analyses, but were unable to find splice sites in the full-length helena sequence. Also, although recombination between mRNAs can produce internal deletions , helena sequences are not sufficiently divergent to allow us to infer the origin of a single copy.
Helena appears to be extinct in D. melanogaster, and this recalls the I element, which also disappeared from the D. melanogaster genome in the past, and reinvaded it only recently . The I and helena elements are both LINE-like elements, leading us to wonder whether amplification/loss of copies could be a characteristic of this type of element. Waves of amplification/loss have been observed in humans, where only the youngest L1 subfamily is active, perhaps as a result of competition between different L1 subfamilies [2, 7].
Our data show that helena has been almost entirely removed from the D. melanogaster genome, and was not subjected to the recent wave of transpositions reported for other elements . In D. simulans, we did observe an insertion site polymorphism of helena, but this corresponds to copies that are being internally deleted by an efficient mechanism. This may be generalized on the basis of data on the LTR retrotransposons 412 and tirant, which have also internal deletions [28, 29]. We still do not clearly understand which mechanisms lead to a low copy number in the D. simulans genome, but a mechanism promoting internal deletions could be a major force at work .
TEs are major players in genome evolution, and the way they are controlled by the host genome is one of the most fundamental questions in evolutionary genomics. Here we show that two closely related species of drosophila have a TE family at different stages in its life cycle. The mechanism by which this is achieved in D. simulans implies that a very efficient internal deletion mechanism is acting on TEs, which is more powerful than the simple neutral evolution of non-active elements. The difference in the amount of TEs between D. melanogaster and D. simulans could be explained by such a process, that doesn't seem to be very active in D. melanogaster present populations.
We worked on fly samples collected from several geographically-distinct, natural populations (confer each Method for natural populations investigated). These populations were maintained in the laboratory as isofemale lines or small mass cultures with around 50 pairs in each generation.
In situ hybridization
Polytene chromosomes from salivary glands of third-instar female larvae were prepared and treated with nick-translated, biotinylated DNA probes, as previously described . Insertion sites were visible as brown bands resulting from a dye-coupled reaction with peroxidase substrate and diaminobenzidine. The insertion site numbers of the TE(s) were determined on all the long chromosomes arms (X, 2L, 2R, 3L, 3R), and were summed to give the total number of labeled sites per diploid genome. We did not take into account the insertions located in pericentromeric regions 20, 40, 41, 80, and 81, because TE site number estimations in these regions are difficult and not reliable for all chromosomes or all squashes. We used a probe (1278 bp) from helena of D. sechellia (AF012044). The following populations of D. melanogaster were investigated: Portugal (Chicharo), Saudi Arabia, Congo (Brazzaville), Reunion Island, Argentina (Virasoro), Bolivia, China (Canton), Vietnam, and Iso line. The D. simulans populations analyzed were from France (Valence), Russia (Moscow), Kenya (Makindu), Zimbabwe, Reunion Island, Australia (Eden, Cann River and Canberra), French Polynesia (Papeete), New Caledonia (Amieu).
DNA was extracted from one or five adult females by a standard phenol-chlorophorm-salt method with proteinase K digestion. The D. melanogaster populations analyzed were from Bolivia, Congo (Brazzaville), China (Canton), Portugal (Chicharo), Reunion Island, Saudi Arabia, Argentina (Virasoro), Vietnam, and ISO line. The D. simulans populations analyzed were from New Caledonia (Amieu), Australia (Eden, Cann River and Canberra), France (Valence), French Polynesia (Papeete), Russia (Moscow), Kenya (Makindu), Zimbabwe, and Reunion Island. The DNA was cut using the Hind III enzyme, which has no restriction site within the helena sequence, and therefore allowed us to estimate the number of complete helena copies. Electrophoresis of a 0.8% agarose gel containing digested DNA was carried out for 17 h. The DNA was denatured (NaOH 0.5 M), and then transferred overnight to a Hybond-N+ nylon membrane. Pre-hybridization and hybridization were carried out at 67°C using a Denhardt 5× solution. The probe used for hybridization (AF012044) was radiolabeled with 32P, using a random procedure from Amersham.
Amplification of ORF1 and ORF2
DNA was extracted from single flies by a standard phenol-chlorophorm method. The following populations of D. melanogaster were investigated: France (Valence and Saint Cyprien), Portugal (Chicharo), Saudi Arabia, Senegal, Congo (Brazzaville), Reunion Island, Guadeloupe, Argentina (Virasoro), Bolivia, and China (Canton). The D. simulans populations analyzed were from France (Valence), Russia (Moscow), Egypt (Tanta), Congo (Brazzaville), Kenya (Meru, Kwalé and Makindu), Zimbabwe, Tanzania (Arusha), Puerto Rico, Japan, Australia (Eden, Cann River and Canberra), French Polynesia (Papeete), Saint Martin, Hawaii, New Caledonia (Amieu), and Portugal (Madeira).
PCR was run using 1 μg DNA with the two following primers – ORF1: H1for (285 5' AAC TGT AAA ATG GAT ACG AAC A 3' 306), H1rev (1808 5' GCC ACT TCA TAA ATT GTT CC 3' 1827). – ORF2: Hel2F (2325 5' CCG GGC TGG GCG ATA TGG 3' 2342), Hel2R (4548 CGT ACA TAC CAG GGG CAG TTG G 3' 4569). PCR was run in 30 cycles with annealing temperatures of 57°C (ORF1) and 56°C (ORF2). We used Euroblue taq from Eurobio. DNA amplified fragments were purified and cloned on competent bacteria (Qiagen kits). Four primers were used for sequencing: M13 forward and reverse; Seq1 (5' CTC TTC CTT CAT TTG GTA CG 3') and Seq2 (5' AAG GGG AAA CAG TGA GAA TA 3') for the complete ORF1; Seq3F (5' TTA GAC CAT GCT CTC GGT TA 3') and Seq3R (5' TGT CAA TTC CTG GAG CTT TA 3') for a fragment of ORF2. Sequencing was performed by Genome Express. Accession numbers (Genbank) from EU168807 to EU168844 correspond to ORF1 fragments. Accession numbers (Genbank) from EU170377 to EU170431 correspond to ORF2 fragments.
Total RNA was extracted from four adult females, four adult males, 10 ovaries and 10 testes from D. simulans populations (France (Valence), Congo (Brazzaville), Kenya (Makindu), Zimbabwe, Australia (Canberra), New Caledonia (Amieu), Portugal (Madeira), United States (San Antonio, San Diego, Arena, SW3)) with the RNeasy protect mini kit from Qiagen. RNA extracts were treated with the Ambion's DNA-free kit. ThermoScript RT-PCR system from Invitrogen was used to synthesize four different cDNA pools (55°C for 90 min and 85°C for 5 min): a control reaction with no retrotranscriptase to test DNA contamination, a pool of total cDNA synthesized with oligo-dt primers, two specific cDNA pools obtained with H1R (ORF1) and Hel2R (ORF2), respectively, corresponding to helena transcripts. All four cDNA pools were tested for the presence of actin cDNA (house keeping gene) by PCR with Act5cfw (5'ATGTGACGAAGAAGTTG3') and Act5cRv (5'TTAGAAGCACTTGCGGTGCA3') primers. Oligo-dt and specific helena cDNA pools were analyzed by PCR using ORF1 and ORF2 specific primers (H1R/H1F and Hel2R/Hel2F).
Total RNA was extracted from adult females or embryos from several D. simulans populations (Valence, Makindu, Amieu, Brazzaville) with the RNeasy protect mini kit from Qiagen. Total RNA extracts were treated with the Ambion's DNA-free kit. Electrophoresis (MOPS, formaldehyde gel) was run for 3 h after RNA denaturing. After washing (water and NaOH, 75 mM) RNA was passively transferred to a nylon membrane, and cross linked for 2 hours at 64°C. Blots were pre-hybridized in hybridization buffer, then hybridized overnight at 42°C in hybridization buffer containing a 32P-labeled helena cDNA probe. The radiolabeled cDNA probe was prepared using a Megaprime DNA Labeling Kit according to the manufacturer's protocol (Cat # RPN 1607; Amersham Biosciences, Little Chalfont, Buckinghamshire, England). Following hybridization, blots were washed in 2 × SSC/0.1% SDS at 42°C and then exposed to X-ray film (KODAK).
Identification of helena copies in the complete genomes
We retrieved the sequences of the chromosome arms 2L, 2R, 3L, 3R, 4, X and the unassigned part (named U) corresponding to the first release of the mosaic assembly of the genome of D. simulans available at the ftp site of the Genome Sequencing Center at the Washington University Medical School . This mosaic assembly corresponds to different strains of D. simulans. We also used the sequenced genome of D. melanogaster . We will refer to the helena copies found in the genomes according to the chromosome name and the start position of the copy (for example chr2L_133500 corresponds to a copy found on the 2L chromosome, and it starts at position 133500).
The helena element was only found in the databases as fragments of the reverse transcriptase (RT). We retrieved the longest sequences from D. yakub a (accession number in Genbank AF012049), D. melanogaster (AF012030) and D. virilis (U26847) to build a chimeric, 1532-bp sequence. Using this chimeric element we searched for copies in the D. simulans sequenced genome using blastn . The reconstructed helena sequence (ID Helena_DS) is available in Repbase . Only matches with an e-value of less than 10e-10 have been retained, and any separated by distances of less than 300 bp have been merged. As the query used corresponds to a small portion of the ORF2, in order to search for longer sequences of helena, we retrieved the matches after adding 5000 bp around their positions. We then performed multiple alignments of these sequences using clustalw  in order to detect the longest copies. By this procedure, we identified a sequence on the chromosome 3R that was the longest of the matches detected. The prediction of potentially coding parts was made using the ORF finder program available on the NCBI web site , and this allowed us to identify two ORFs. It was not possible to use the presence of target site duplication to determine the exact position of the beginning of the sequence, because the copy was surrounded by unidentified bases, and so we performed a blast search in the draft sequence of D. sechellia, the closest relative to D. simulans. This allowed us to find a homologous copy, and to identify the beginning of the complete copy of helena. Once this copy had been identified, it was used as a query to perform blast searches in the D. simulans and D. melanogaster genomes to determine the helena copy populations.
The computation of the percentage identity was performed using the DNADIST program in the PHYLIP package . We used the sequence editor Seaview  to visualize the sequences and the alignments. Splice sites and transcription binding sites were predicted by the Softberry tools  and Genomatix ; PEPcoil ( allowed us to find the coiled coil domain in ORF 1. Conserved domains in both ORF1 and ORF2 were predicted with the "Conserved domain search" tool from NCBI. Sequenced copies were aligned with T_coffee . Phylogenetic analysis were made using maximum likelihood with HKY substitution model implemented in PhyML . The reconstruction was performed on the cloned DNA sequences of the ORF1 and ORF2 region from the different populations of D. simulans, and from some sequences detected in the sequenced genome (we eliminated sequences that were too short relative to the global length of the alignment).
Age was estimated using the Bowen and McDonald method  with the formula Age = K/(2r), where K is the divergence between the two copies calculated from the Kimura two-parameter distance via DNAdist, and r is the synonymous substitution rate per site per million years in D. melanogaster (r = 0.016 from Li ). It is important to note that the age of helena copies is underestimated due to the lack of knowledge about conversion and substitution rates in D. melanogaster genome, and is also unreliable when applied to old and highly diverged copies.
dead on arrival
long interspersed nuclear element
long terminal repeat
open reading frame
We thank Monika Ghosh for reviewing the English text. This work was funded by the Centre National de la Recherche Scientifique (UMR 5558) and the IMPBio program.
- Biemont C, Vieira C: Genetics: junk DNA as an evolutionary force. Nature. 2006, 443 (7111): 521-524. 10.1038/443521a.PubMedView ArticleGoogle Scholar
- Khan H, Smit A, Boissinot S: Molecular evolution and tempo of amplification of human LINE-1 retrotransposons since the origin of primates. Genome research. 2006, 16 (1): 78-87. 10.1101/gr.4001406.PubMedPubMed CentralView ArticleGoogle Scholar
- Lander ES, Linton LM, Birren B, Nusbaum C, Zody MC, Baldwin J, Devon K, Dewar K, Doyle M, FitzHugh W: Initial sequencing and analysis of the human genome. Nature. 2001, 409 (6822): 860-921. 10.1038/35057062.PubMedView ArticleGoogle Scholar
- Eickbush TH, Furano AV: Fruit flies and humans respond differently to retrotransposons. Curr Opin Genet Dev. 2002, 12 (6): 669-674. 10.1016/S0959-437X(02)00359-3.PubMedView ArticleGoogle Scholar
- Bennetzen JL: Transposable elements, gene creation and genome rearrangement in flowering plants. Current opinion in genetics & development. 2005, 15 (6): 621-627. 10.1016/j.gde.2005.09.010.View ArticleGoogle Scholar
- Vitte C, Bennetzen JL: Analysis of retrotransposon structural diversity uncovers properties and propensities in angiosperm genome evolution. Proc Natl Acad Sci USA. 2006, 103 (47): 17638-17643. 10.1073/pnas.0605618103.PubMedPubMed CentralView ArticleGoogle Scholar
- Boissinot S, Furano AV: The recent evolution of human L1 retrotransposons. Cytogenet Genome Res. 2005, 110 (1–4): 402-406. 10.1159/000084972.PubMedView ArticleGoogle Scholar
- Chambeyron S, Bucheton A: I elements in Drosophila: in vivo retrotransposition and regulation. Cytogenetic and genome research. 2005, 110 (1–4): 215-222. 10.1159/000084955.PubMedView ArticleGoogle Scholar
- SanMiguel P, Gaut BS, Tikhonov A, Nakajima Y, Bennetzen JL: The paleontology of intergene retrotransposons of maize. Nature genetics. 1998, 20 (1): 43-45. 10.1038/1695.PubMedView ArticleGoogle Scholar
- Li YJ, Satta Y, Takahata N: Paleo-demography of the Drosophila melanogaster subgroup: application of the maximum likelihood method. Genes & genetic systems. 1999, 74 (4): 117-127. 10.1266/ggs.74.117.View ArticleGoogle Scholar
- Vieira C, Lepetit D, Dumont S, Biemont C: Wake up of transposable elements following Drosophila simulans worldwide colonization. Mol Biol Evol. 1999, 16 (9): 1251-1255.PubMedView ArticleGoogle Scholar
- Biemont C, Nardon C, Deceliere G, Lepetit D, Loevenbruck C, Vieira C: Worldwide distribution of transposable element copy number in natural populations of Drosophila simulans. Evolution Int J Org Evolution. 2003, 57 (1): 159-167.View ArticleGoogle Scholar
- Petrov DA, Hartl DL: High rate of DNA loss in the Drosophila melanogaster and Drosophila virilis species groups. Molecular Biology and Evolution. 1998, 15 (3): 293-302.PubMedView ArticleGoogle Scholar
- Lerat E, Rizzon C, Biemont C: Sequence divergence within transposable element families in the Drosophila melanogaster genome. Genome Res. 2003, 13 (8): 1889-1896.PubMedPubMed CentralGoogle Scholar
- Arkhipova IR, Lyubomirskaya NV, Ilyn YV: Drosophila Retrotransposons. 1995, Berlin: SpringerGoogle Scholar
- Assembly/Alignement/Annotation of 12 relatedDrosophila species. [http://rana.lbl.gov/drosophila/index.html]
- Malik HS, Burke WD, Eickbush TH: The age and evolution of non-LTR retrotransposable elements. Molecular biology and evolution. 1999, 16 (6): 793-805.PubMedView ArticleGoogle Scholar
- Hohjoh H, Singer MF: Cytoplasmic ribonucleoprotein complexes containing human LINE-1 protein and RNA. Embo J. 1996, 15 (3): 630-639.PubMedPubMed CentralGoogle Scholar
- Pardue ML, Danilevskaya ON, Lowenhaupt K, Wong J, Erby K: The gag coding region of the Drosophila telomeric retrotransposon, HeT-A, has an internal frame shift and a length polymorphic region. J Mol Evol. 1996, 43 (6): 572-583. 10.1007/BF02202105.PubMedView ArticleGoogle Scholar
- Casavant NC, Scott L, Cantrell MA, Wiggins LE, Baker RJ, Wichman HA: The end of the LINE?: lack of recent L1 activity in a group of South American rodents. Genetics. 2000, 154 (4): 1809-1817.PubMedPubMed CentralGoogle Scholar
- Rohrmann GF, Karplus PA: Relatedness of baculovirus and gypsy retrotransposon envelope proteins. BMC Evol Biol. 2001, 1: 1-10.1186/1471-2148-1-1.PubMedPubMed CentralView ArticleGoogle Scholar
- Fablet M, Rebollo R, Biemont C, Vieira C: The evolution of retrotransposon regulatory regions and its consequences on the Drosophila melanogaster and Homo sapiens host genomes. Gene. 2007, 390 (1–2): 84-91. 10.1016/j.gene.2006.08.005.PubMedView ArticleGoogle Scholar
- Lozovskaya ER, Nurminsky DI, Petrov DA, Hartl DL: Genome size as a mutation-selection-drift process. Genes Genet Syst. 1999, 74 (5): 201-207. 10.1266/ggs.74.201.PubMedView ArticleGoogle Scholar
- Brookfield JF: Evolutionary forces generating sequence homogeneity and heterogeneity within retrotransposon families. Cytogenet Genome Res. 2005, 110 (1–4): 383-391. 10.1159/000084970.PubMedView ArticleGoogle Scholar
- Belancio VP, Hedges DJ, Deininger P: LINE-1 RNA splicing and influences on mammalian gene expression. Nucleic Acids Res. 2006, 34 (5): 1512-1521. 10.1093/nar/gkl027.PubMedPubMed CentralView ArticleGoogle Scholar
- Roy SW, Penny D: Widespread intron loss suggests retrotransposon activity in ancient apicomplexans. Molecular biology and evolution. 2007, 24 (9): 1926-1933. 10.1093/molbev/msm102.PubMedView ArticleGoogle Scholar
- Bucheton A, Vaury C, Chaboissier MC, Abad P, Pelisson A, Simonelig M: I elements and the Drosophila genome. Genetica. 1992, 86 (1–3): 175-190. 10.1007/BF00133719.PubMedView ArticleGoogle Scholar
- Fablet M, McDonald JF, Biemont C, Vieira C: Ongoing loss of the tirant transposable element in natural populations of Drosophila simulans. Gene. 2006, 375: 54-62. 10.1016/j.gene.2006.02.008.PubMedView ArticleGoogle Scholar
- Mugnier N, Biemont C, Vieira C: New regulatory regions of Drosophila 412 retrotransposable element generated by recombination. Molecular biology and evolution. 2005, 22 (3): 747-757. 10.1093/molbev/msi060.PubMedView ArticleGoogle Scholar
- Vieira C, Biemont C: Transposable element dynamics in two sibling species: Drosophila melanogaster and Drosophila simulans. Genetica. 2004, 120 (1–3): 115-123. 10.1023/B:GENE.0000017635.34955.b5.PubMedView ArticleGoogle Scholar
- Biemont C, Monti-Dedieu L, Lemeunier F: Detection of transposable elements in Drosophila salivary gland polytene chromosomes by in situ hybridization. Methods Mol Biol. 2004, 260: 21-28.PubMedGoogle Scholar
- Genome Sequencing Center at the Washington University Medical School. [http://hgdownload.cse.ucsc.edu/downloads.html#droSim]
- Ensembl Genome Browser. [http://www.ensembl.org/index.html]
- Karlin S, Altschul SF: Methods for assessing the statistical significance of molecular sequence features by using general scoring schemes. Proc Natl Acad Sci USA. 1990, 87 (6): 2264-2268. 10.1073/pnas.87.6.2264.PubMedPubMed CentralView ArticleGoogle Scholar
- Repbase. [http://www.girinst.org/]
- Thompson JD, Higgins DG, Gibson TJ: CLUSTAL W: improving the sensitivity of progressive multiple sequence alignment through sequence weighting, position-specific gap penalties and weight matrix choice. Nucleic Acids Res. 1994, 22 (22): 4673-4680. 10.1093/nar/22.22.4673.PubMedPubMed CentralView ArticleGoogle Scholar
- ORF Finder. [http://www.ncbi.nlm.nih.gov/gorf/gorf.html]
- Felsenstein J: An alternating least squares approach to inferring phylogenies from pairwise distances. Syst Biol. 1997, 46 (1): 101-111. 10.2307/2413638.PubMedView ArticleGoogle Scholar
- Galtier N, Gouy M, Gautier C: SEAVIEW and PHYLO_WIN: two graphic tools for sequence alignment and molecular phylogeny. Comput Appl Biosci. 1996, 12 (6): 543-548.PubMedGoogle Scholar
- Softberry tools. [http://www.softberry.com/berry.phtml]
- Genomatix. [http://www.genomatix.de]
- Lupas A, Van Dyke M, Stock J: Predicting coiled coils from protein sequences. Science. 1991, 252 (5010): 1162-1164. 10.1126/science.252.5009.1162.PubMedView ArticleGoogle Scholar
- Notredame C, Higgins DG, Heringa J: T-Coffee: A novel method for fast and accurate multiple sequence alignment. J Mol Biol. 2000, 302 (1): 205-217. 10.1006/jmbi.2000.4042.PubMedView ArticleGoogle Scholar
- Guindon S, Gascuel O: A simple, fast, and accurate algorithm to estimate large phylogenies by maximum likelihood. Systematic biology. 2003, 52 (5): 696-704. 10.1080/10635150390235520.PubMedView ArticleGoogle Scholar
- Bowen NJ, McDonald JF: Drosophila euchromatic LTR retrotransposons are much younger than the host species in which they reside. Genome research. 2001, 11 (9): 1527-1540. 10.1101/gr.164201.PubMedPubMed CentralView ArticleGoogle Scholar
- Li W: Molecular Evolution. 1997, Sunderland, MA: Sinauer AssociatesGoogle Scholar
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.