- Research article
- Open Access
Effects of Alu elements on global nucleosome positioning in the human genome
BMC Genomics volume 11, Article number: 309 (2010)
Understanding the genome sequence-specific positioning of nucleosomes is essential to understand various cellular processes, such as transcriptional regulation and replication. As a typical example, the 10-bp periodicity of AA/TT and GC dinucleotides has been reported in several species, but it is still unclear whether this feature can be observed in the whole genomes of all eukaryotes.
With Fourier analysis, we found that this is not the case: 84-bp and 167-bp periodicities are prevalent in primates. The 167-bp periodicity is intriguing because it is almost equal to the sum of the lengths of a nucleosomal unit and its linker region. After masking Alu elements, these periodicities were greatly diminished. Next, using two independent large-scale sets of nucleosome mapping data, we analyzed the distribution of nucleosomes in the vicinity of Alu elements and showed that (1) there are one or two fixed slot(s) for nucleosome positioning within the Alu element and (2) the positioning of neighboring nucleosomes seems to be in phase, more or less, with the presence of Alu elements. Furthermore, (3) these effects of Alu elements on nucleosome positioning are consistent with inactivation of promoter activity in Alu elements.
Our discoveries suggest that the principle governing nucleosome positioning differs greatly across species and that the Alu family is an important factor in primate genomes.
The genomic DNA of eukaryotes forms chromatin structures with several proteins. Chromatin is composed of nucleosome cores in which 146-147 base pairs (bp) of DNA are wrapped in 1.67 turns around a histone octamer containing two copies each of four core histones: H2A, H2B, H3, and H4 . Another histone (linker histone) binds to about 20 bp of DNA in the linker region flanking the nucleosome core [2, 3]. Nucleosomes are involved in various cellular processes, including transcription, because chromatin can limit the accessibility of regulatory sites. For example, it has been reported in several organisms that the nucleosome occupancy rate upstream from transcription start sites (TSSs) is lower than that in other regions [4–12]. Therefore, understanding the mechanism of nucleosome positioning is important for the analysis of transcriptional regulation and promoter functions.
It is known that nucleosome positioning can be affected by DNA sequence. Many previous studies have identified various motifs for nucleosome positioning or inhibition with in vivo and in vitro experiments [13–18]. It is also known that 10-bp periodic AA/TT or GC dinucleotides are strongly associated with nucleosome positioning in the genomes of several species and in synthetic DNAs [19–22]. Short oligonucleotides occurring at intervals of about 10 bp are associated with the positions of the major grooves or minor grooves facing the histone surface and with the bendability of DNA during nucleosome formation . Using these dependencies, some researchers recently succeeded, more or less, in the computational prediction of nucleosome positions in the genome sequences of several yeasts [24–27]. In particular, Segal et al. explained about 50% of in vivo nucleosome positions using a position weight matrix of center-aligned mononucleosome DNA in budding yeast and chicken . The 10-bp periodicity has been observed by Fourier analysis in the genome of nematode, plant, insect and fungus .
In recent years, high-throughput sequencing techniques and tiling array experiments have provided an avalanche of nucleosomal DNA location information in the human [8–10], fly [11, 30], nematode [7, 20], and budding yeast genomes [4–6, 12]. Schones et al. demonstrated nucleosomal reorganization during the activation of human T cells using a large number of nucleosomal DNAs, which were massively sequenced with a new-generation sequencer. Lee et al. and Shivaswamy et al. showed that about 70%-80% of the whole genome of budding yeast is occupied by nucleosomes. These large-scale experiments make it possible to analyze the sequence dependencies of global nucleosomal positioning across a wide range of organisms.
In this study, we first asked whether the reported periodic motifs can widely affect in vivo nucleosome locations through the whole genomes of all eukaryotes. Using Fourier analysis, the spectrum of primate genomes does not exhibit clear peaks with a 10-bp periodicity: strong and wide 84-bp and 167-bp periodicities are observed, instead. These periodicities, which may be associated with the length of DNA wrapping core histones and the linker histone, mainly originate from Alu repetitive elements, as their strength decreased markedly in Alu-masked genomes.
The Alu family are primate-specific short interspersed elements (SINEs), and constitute the most prevalent repetitive element in the human genome . Alu elements are categorized into two groups: monomers and dimers. A typical dimeric Alu is about 300 bp long, and is composed of two distinct GC- and CpG-rich monomers flanking an A-rich region and a poly(A) tract. Monomeric Alu elements consist of two classes: free left Alu monomers (FLAM) and free right Alu monomers (FRAM), corresponding to each monomer in a dimer. The left monomer is slightly shorter than the right one . Although a few Alu elements in promoters are reported to affect their downstream gene expression [33, 34], most of them are silent in cells. Thus, specific positioning of nucleosomes on Alu elements may be important in masking unnecessary effects of Alu's to nearby genes. DNase I nicking analyses have demonstrated that several dimeric Alu elements have some affinity to core histones [35, 36]. According to these studies, two nucleosomes are formed in both sides of the central A-tract of Alu elements.
Using large-scale nucleosome mapping data, we observed that such specific positioning occurs globally in the entire genome. We further showed that nucleosomes are also arranged in nucleosomal repeat lengths (about 170-200 bp) around them. Our discoveries should be useful in the prediction of nucleosomal positions in primates and the analysis of transcriptional regulation.
Genome-wide nucleotide periodicity
We analyzed the genome-wide nucleotide periodicity in 16 different species (See additional file 1) under the assumption that if the 10-bp periodic nucleotides are the main factor determining nucleosome positioning, peaks of this periodicity should also be observed in the whole genome. The strength of the periodicity was calculated for 12 kinds of mono- and di-nucleotide steps using Fourier analysis [21, 37].
In consistent with a previous study , clear spikes with a periodicity of about 10 bp or 11 bp were observed in fishes, chordates, an insect, a nematode, plants, and a fungus with the AA/TT dinucleotide step (Figure 1). In the nematode genome, another small peak with a periodicity of about 9 bp was observed (See additional file 2). The spectra of these organisms calculated with other nucleotide steps also showed clear peaks of about 9-bp, 10-bp, or 11-bp periodicity. In the chicken genome, weak peaks of 10-bp periodicity were observed only for the A/T and G/C steps. However, no clear peaks with these periodicities were observed in mammals. In contrast, two large and wide peaks centered at about 84 bp and 167 bp were observed in the human, chimpanzee, and rhesus genomes. These primate-specific peaks were clearly observed in the AA/TT, A/T and G/C steps, and were especially remarkable in the AA/TT step (See additional file 3). The value of 167 bp corresponds approximately to the sum of the length of a nucleosome core (147 bp) and the length of the linker-histone-binding region (20 bp), and 84 bp corresponds to about half this length. This observation suggests that these periodicities are related to nucleosome positioning in primate genomes.
Because it is known that some repetitive elements are detectable by nucleotide periodicities , we next analyzed the genome-wide periodicity while masking all Alu elements, which are primate-specific SINEs detected by RepeatMasker. The strengths of the 84-bp and 167-bp periodicities in the Alu-masked primate genomes were remarkably lower than those in the nonmasked genomes (green lines in Figure 1 and additional file 3). Although weak and sharp peaks of 84-bp or 167-bp periodicity still remained in some nucleotide steps, they were possibly derived from Alu elements that had not been identified by RepeatMasker or from some other genome features. Thus, it is clear that these 84-bp and 167-bp periodicities mainly originate from Alu repetitive elements.
Effects of Alu elements on nucleosome positioning
To confirm the relationship between Alu elements and nucleosome positioning in the human genome, we analyzed the distribution of nucleosomes within and around the Alu elements. In this study, the Alu family was categorized into three classes: dimer, FLAM, and FRAM. After removing incomplete Alu elements, we identified 763,485 dimers of 280-320 bp in length, 47,815 FLAMs of 110-150 bp, and 17,255 FRAMs of 150-190 bp (Figure 2A). These occupy about 7.42%, 0.20% and 0.09% of the whole human genome, respectively.
We used the data of paired-end nucleosomal DNA tags (sequenced fragments) from HEK293 cells made by the micrococcal nuclease (MNase) digestion and by the sequencing with the Illumina GA-II sequencers (Irie et al., submitted). In total, 27,756,155 paired-end nucleosome DNA tags were mapped on the human genome (Table 1). More than 90% (26,340,652 tags) of them showed unique positions, and about 5.91% (1,639,194 tags) were assigned within the Alu elements. By aligning the nucleosome signal (i.e., the smoothed positional distribution of mapped tag frequency; see Methods) to the central position of each type of Alu elements, we found one clear peak on the left side and another weaker peak on the right side in dimeric Alu elements (Figure 2B) as well as a single clear peak in both FLAMs and FRAMs (Figure 2C and 2D, respectively). On the other hand, large troughs of the nucleosome signal were observed near the A-rich regions (See additional file 4). In the dimeric Alu elements, the signal intensity of the left peak is not so different from that of randomly extracted fragments (used as control) and the intensity of the right peak is much smaller than the normal level. These results indicate that the positions where the nucleosome structure is formed within dimeric Alu elements are very limited; of the two possible slots, one is used at the normal level while the other is disfavored. On the other hand, monomeric Alu elements have a single possible slot.
The 181,551 multi-hit tags that overlap with Alu elements were not included in the above result (Table 1). For about a half of them (95,382 tags), all of their multiple hits were mapped within Alu elements while for 80% of them (146,477 tags) more than 85% of their multiple hits overlapped with Alu elements (Figure 3). Then, from the above result only, there may remain some concern that the observed slots are only artifacts caused by the removal of tags mapped to multiple locations. Thus, we randomly chose one from each of multi-hit tags that were mapped within the Alu region and redrew the distribution of nucleosome signal around Alu elements (Additional file 5). Similarly with Figures 2B-D, the nucleosome distribution shows two or one slots in Alu elements and lower occupancy of nucleosome is observed in the right arm of the dimeric Alu's. When we repeated the same procedure using the muti-hit tags more than 85% of which overlap with Alu elements, similar distributions were observed (Additional file 5). Furthermore, standard deviation of the relative distances of multiple hits from the center of nearest Alu elements for each tag was only 2.248 bp on average. Overall, we concluded that the nucleosome slots in Alu elements are not artifacts.
We also detected phased nucleosome positioning at approximately the nucleosome repeat length (about 170-200 bp) around the Alu elements (yellow ovals in Figure 2) . This phased frequency extended to both orientations and became weaker as the site is more distant from Alu elements. These observations suggest that Alu elements contain nucleosomes in specific positions, and also influence the positioning of neighboring nucleosomes.
Validation of the positioning of neighboring nucleosomes by independent data
To verify this suggestion with another independent experiment, we analyzed the distribution of nucleosome locations using the data from high-resolution tiling arrays for 3,962 human promoters in seven different cell types . Each probe in every array was aligned by both edges of the Alu elements, including both monomers and dimers, and the signals were averaged at each position for all arrays. The hybridization signals were significantly higher than the background signal at regions just upstream and downstream from Alu elements (Figure 4A). This result indicates that nucleosomes are preferentially located in the neighborhood of Alu elements. This conclusion remains unchanged in the data for each cell type, except A375 (See additional file 6). Furthermore, in a region of about 100 bp immediately upstream and downstream from the Alu elements, the signals were lower than the background signal. This tendency was also observed in the distribution of nucleosome centers (Figure 2B-D). These results imply that the regions immediately upstream and downstream from Alu elements are likely to be preferentially used as linker regions. Although we analyzed the signals flanking other repetitive elements, there was little difference from the background signal (Figure 4B and additional file 6), indicating that the effect on the positioning of neighboring nucleosomes is specific to Alu elements.
Considering these data together, it is clear that the Alu family significantly affects nucleosome positioning in the human genome.
Relationship between nucleosome positioning and gene expression
It has been suggested that nucleosomes are predominant in promoters of unexpressed genes [8, 9]. Therefore, the observed restriction of nucleosome positioning within and around Alu elements may influence their promoter functions in vivo. To verify this possibility, we calculated the average expression rate from the number of precise 5'-end cDNA tags mapped within Alu elements. As controls, the rates for 5'-end tags mapped in regions around RefSeq TSSs and randomly selected regions were also calculated. Precise 5'-end tags for HEK293 and MCF7 cells were previously detected by the oligo-capping method and were sequenced with an Illumina Solexa sequencer . The average expression rates in an Alu element were about 0.045 and 0.062 parts per million (p.p.m) in each cell type, respectively (Figure 5). In contrast, the expression rates in RefSeq TSSs were more than 20 (24.09 and 26.13 p.p.m, respectively), remarkably higher than those in the Alu elements, and those at random sites were also higher than those in Alu elements (1.16 and 1.62 p.p.m, respectively). We further calculated the rates in the flanking regions: [-900, -601], [-600, -301], [-300-1], [+1, +300], [+301, +600] and [+601, +900]; -1 and +1 indicate 5' and 3' end of Alu elements, respectively. The expression rates at the flanking regions are slightly higher than those in Alu elements (from 0.099 to 0.276 p.p.m in HEK293 and from 0.128 to 0.270 p.p.m in MCF7), but are significantly lower than those at random sites. These results suggest that most Alu elements do not have the activity of promoter.
Alu elements are distributed only in primates, and comprise about 10% of the whole human genome . In this study, we showed that nucleosome positioning is significantly influenced within and around Alu elements using large-scale nucleosome mapping data. Englander et al. previously reported that dimeric Alu elements have a capacity containing two nucleosomes [35, 36]. These positions are consistent with the two peaks observed in Figure 2B. Since DNase I nicking pattern in their experiment is less clear in the right arm compared with the left arm of dimeric Alu elements, the low occupancy in the right arm observed in our analysis may be caused by the lower stability of nucleosome positioning. From a massive number of nucleosomal DNA sequence data, we demonstrated that neighboring nucleosomes tend to be arranged with regular intervals. Nucleosome signals from the tiling array data showed some preference for nucleosome positioning just around Alu elements. The A-rich sequences observed in low nucleosome density regions are known as a motif for inhibiting nucleosome formation . From our analysis based on two independent data sets, we conclude that the lower nucleosome signals at the boundary of Alu elements affect the arrangement of nucleosome positioning around them. Although nucleosome depletions are often observed in the promoters of active genes, few TSS tags could be mapped in Alu elements and their flanking regions. It is possible that restriction of Alu elements is regulated by other epigenetic factors. This hypothesis is supported by two previous reports that 76.2% of CpG sites in Alu elements are completely methylated , and that methylation of H3 lysine 9 is enriched in Alu elements .
The genome-wide periodicity of 16 organisms showed differences in their sequence dependence. Peaks with 10-bp periodicity were observed in organisms from budding yeast to chicken. Our results are in agreement with those of Segal et al., who showed that the nucleosome locations in budding yeast can be predicted with the model constructed from chicken nucleosomal DNA. In some organisms, periodicities of about 9 bp and 11 bp have been found. These periodicities might be related to the minimum and maximum periods of the double helix of DNA in nucleosomes because its observed value varies from 9.4 bp to 10.9 bp . Furthermore, Gupta et al. previously showed 3-bp periodicities of CG and GC dinucleotides are overrepresented in nucleosome-forming sequences in promoters and ENCODE regions . In our results, peaks of CG 3-bp periodicities are found in many species, but not in primates, suggesting that these sequence dependencies may not effect across the whole primate genomes.
It is surprising that the sequence features governing global nucleosomal positioning are quite different among organisms, even though the core histone protein families are highly conserved among species . Although it has been reported that a set of DNA molecules with the highest affinity with the histone octamer in an in vitro selection assay showed a 10-bp periodicity of mono- or dinucleotide steps , our result suggests that they may not use these features as the major mechanism of nucleosomal positioning, to allow flexibility of chromatin remodeling and complex transcription regulation. We showed that a significant part of nucleosome positioning in the primate genomes can be explained by 84-bp and 167-bp periodicities, which were previously reported in human chromosomes 21 and 22 by a similar method . Here, we confirmed that these periodicities are specific to primates because they are due to primate-specific Alu elements.
Overall, our study provides an important clue to understanding the whole chromatin composition of the human genome. We hope that our discoveries will extend our understanding of the nucleosomal organization in primate genomes, and contribute essential knowledge about the complexities of transcriptional regulation.
Collection of genome sequences and nucleosome mapping data
Genome sequences were downloaded from UCSC, The institute for Genomic Research (TIGR), RIKEN, and Saccharomyces genome database (SGD) (See additional file 1). All positions of repetitive elements and RefSeq genes were obtained from "rmsk" files and the "refGene.txt" file in the UCSC database, respectively.
The tiling array data for human promoters (GSE6385) were downloaded from Gene Expression Omnibus http://www.ncbi.nlm.nih.gov/geo/. About 40 million raw sequence reads of precise TSSs from HEK293 and MCF7 cells were obtained from DBTSS http://dbtss.hgc.jp/.
Fourier analysis of DNA sequences
For each species, 10,000 fragments of length 8,193 (213 + 1) bp were randomly extracted from the whole-genome sequence without gap regions ("N" characters). As a control, we generated 10,000 random DNA sequences that had the same base composition as the genome sequence of each organism. To apply discrete Fourier transformations to DNA sequences, we transformed the nucleotide steps to binary codes. For two mononucleotide steps and 10 dinucleotide steps, the target step γ; was converted to 1, and the other steps were converted to 0. For example, if γ is AA/TT, a DNA sequence "CTTGAAT" is changed to the binary sequence "010010".
The power spectrum F γ (n) of the binary sequence B γ (k) (k = 0, 1, ..., N - 1), whose length is N, is defined as follows:
where j2 = -1, n = 0, 1, 2, ..., (N/2) - 1, and W(k) is a window function. A window function was used for noise reduction at high frequency. In this study, we used the Welch window , defined as follows:
To compare the spectra of various genomes, we used the signal-to-noise (S/N) ratio, which is the ratio of each periodicity signal to the background noise of a DNA sequence. The ratio was calculated by the power spectrum F γ (n) as follows:
The background noise is defined as the average power spectrum. The S/N ratio R γ (n) is interpreted as the relative strength of the periodicity p (= N/n) [38, 48, 49]. The S/N ratios were calculated for all DNA fragments, and were averaged for each organism. The Fourier transform was calculated with the FFTW3 library .
Analysis of nucleosome distributions within and around Alu elements
In this study, the Alu family was categorized into three classes: dimer Alu, FLAM, and FRAM, based on the "repName" field (See additional file 7). We also restricted the length of each Alu class to 280-320 bp, 110-150 bp, and 150-190 bp, respectively. Sequences that were longer or shorter than these lengths were discarded.
The paired-end nucleosomal DNA tags were taken from HEK293 cells by the micrococcal nuclease (MNase) digestion and by the sequencing with the Illumina GA-II sequencers (Irie et al., submitted). All 36-bp nucleosome reads were mapped to the human genome (chr1-22, chrX and chrY) using Bowtie (version 0.12.2) with the option: "-f -I 122 -X 172 -n 0 -a --best --strata --chunkmbs 2048" . Because the 5' ends of nucleosomal DNA were sequenced on both strands, their midpoint was presumed to be the positions of the nucleosome core centers. Since the digestion of MNase does not always produce complete 147-bp DNA fragments, we further calculated the nucleosome signal S(i), which is introduced as the "coarse-grain smoothing" in . As background, 30 million 36-bp paired-end genome fragments, whose interval is 147 bp, were randomly extracted and were also mapped to the human genome by Bowtie. In the same way, we deduced the background signal S back (i) from the uniquely mapped random fragments. The signals, S(i) and S back (i), were normalized with the p.p.b. (parts per billion) unit.
Analysis of nucleosome signals from tiling array data
In the human promoter tiling array , we used probes whose center positions were within 600 bp of Alu elements. We also selected other repetitive elements (all repetitive elements except Alu in the UCSC annotation) that were the same size as the Alu elements, and probes within 600 bp of them were extracted similarly. Each probe was sorted by the distance from the 5' end or the 3' end of these repetitive elements. The hybridization values of the probes at each distance were averaged in each cell type or in all cells. As the background of the signals, we shuffled the hybridization values of all probes in the tiling array. This shuffling was repeated 10 times. Averages and standard deviations were calculated from the 10 randomized data sets and were represented by points and error bars, respectively.
Average expression level of genes
All 24-25-bp precise 5'-end cDNA tags were mapped in Alu family regions, corresponding to ± 150 bp from TSSs of 25,892 RefSeq genes and ± 150 bp from 25,892 randomly selected sites 24 bp downstream, using SeqMap (See additional file 8) . The average expression rate was calculated as p.p.m for each category:
To obtain the random sites, we repeated the calculation of this rate 10 times, and calculated the means and standard deviations of the results.
Richmond TJ, Davey CA: The structure of DNA in the nucleosome core. Nature. 2003, 423 (6936): 145-150. 10.1038/nature01595.
Gomez-Marquez J, Rodriguez P: Prothymosin alpha is a chromatin-remodelling protein in mammalian cells. Biochem J. 1998, 333 (Pt 1): 1-3.
An W, van Holde K, Zlatanova J: Linker histone protection of chromatosomes reconstituted on 5S rDNA from Xenopus borealis:a reinvestigation. Nucleic Acids Res. 1998, 26 (17): 4042-4046. 10.1093/nar/26.17.4042.
Lee W, Tillo D, Bray N, Morse RH, Davis RW, Hughes TR, Nislow C: A high-resolution atlas of nucleosome occupancy in yeast. Nat Genet. 2007, 39 (10): 1235-1244. 10.1038/ng2117.
Shivaswamy S, Bhinge A, Zhao Y, Jones S, Hirst M, Iyer VR: Dynamic remodeling of individual nucleosomes across a eukaryotic genome in response to transcriptional perturbation. PLoS Biol. 2008, 6 (3): e65-10.1371/journal.pbio.0060065.
Yuan GC, Liu YJ, Dion MF, Slack MD, Wu LF, Altschuler SJ, Rando OJ: Genome-scale identification of nucleosome positions in S. cerevisiae. Science. 2005, 309 (5734): 626-630. 10.1126/science.1112178.
Valouev A, Ichikawa J, Tonthat T, Stuart J, Ranade S, Peckham H, Zeng K, Malek JA, Costa G, McKernan K, Sidow A, Fire A, Johnson SM: A high-resolution, nucleosome position map of C. elegans reveals a lack of universal sequence-dictated positioning. Genome Res. 2008, 18 (7): 1051-1063. 10.1101/gr.076463.108.
Schones DE, Cui K, Cuddapah S, Roh TY, Barski A, Wang Z, Wei G, Zhao K: Dynamic regulation of nucleosome positioning in the human genome. Cell. 2008, 132 (5): 887-898. 10.1016/j.cell.2008.02.022.
Ozsolak F, Song JS, Liu XS, Fisher DE: High-throughput mapping of the chromatin structure of human promoters. Nat Biotechnol. 2007, 25 (2): 244-248. 10.1038/nbt1279.
Giresi PG, Kim J, McDaniell RM, Iyer VR, Lieb JD: FAIRE (Formaldehyde-Assisted Isolation of Regulatory Elements) isolates active regulatory elements from human chromatin. Genome Res. 2007, 17 (6): 877-885. 10.1101/gr.5533506.
Mavrich TN, Jiang C, Ioshikhes IP, Li X, Venters BJ, Zanton SJ, Tomsho LP, Qi J, Glaser RL, Schuster SC, Gilmour DS, Albert I, Pugh BF: Nucleosome organization in the Drosophila genome. Nature. 2008, 453 (7193): 358-362. 10.1038/nature06929.
Whitehouse I, Rando OJ, Delrow J, Tsukiyama T: Chromatin remodelling at promoters suppresses antisense transcription. Nature. 2007, 450 (7172): 1031-1035. 10.1038/nature06391.
Wang YH, Amirhaeri S, Kang S, Wells RD, Griffith JD: Preferential nucleosome assembly at DNA triplet repeats from the myotonic dystrophy gene. Science. 1994, 265 (5172): 669-671. 10.1126/science.8036515.
Widlund HR, Cao H, Simonsson S, Magnusson E, Simonsson T, Nielsen PE, Kahn JD, Crothers DM, Kubista M: Identification and characterization of genomic nucleosome-positioning sequences. J Mol Biol. 1997, 267 (4): 807-817. 10.1006/jmbi.1997.0916.
Cao H, Widlund HR, Simonsson T, Kubista M: TGGA repeats impair nucleosome formation. J Mol Biol. 1998, 281 (2): 253-260. 10.1006/jmbi.1998.1925.
Morohashi N, Yamamoto Y, Kuwana S, Morita W, Shindo H, Mitchell AP, Shimizu M: Effect of sequence-directed nucleosome disruption on cell-type-specific repression by alpha2/Mcm1 in the yeast genome. Eukaryot Cell. 2006, 5 (11): 1925-1933. 10.1128/EC.00105-06.
Tomita N, Fujita R, Kurihara D, Shindo H, Wells RD, Shimizu M: Effects of triplet repeat sequences on nucleosome positioning and gene expression in yeast minichromosomes. Nucleic Acids Res Suppl. 2002 (2): 231-232.
Shimizu M, Mori T, Sakurai T, Shindo H: Destabilization of nucleosomes by an unusual DNA conformation adopted by poly(dA) small middle dotpoly(dT) tracts in vivo. EMBO J. 2000, 19 (13): 3358-3365. 10.1093/emboj/19.13.3358.
Ioshikhes I, Bolshoy A, Derenshteyn K, Borodovsky M, Trifonov EN: Nucleosome DNA sequence pattern revealed by multiple alignment of experimentally mapped sequences. J Mol Biol. 1996, 262 (2): 129-139. 10.1006/jmbi.1996.0503.
Johnson SM, Tan FJ, McCullough HL, Riordan DP, Fire AZ: Flexibility and constraint in the nucleosome core landscape of Caenorhabditis elegans chromatin. Genome Res. 2006, 16 (12): 1505-1516. 10.1101/gr.5560806.
Satchwell SC, Drew HR, Travers AA: Sequence periodicities in chicken nucleosome core DNA. J Mol Biol. 1986, 191 (4): 659-675. 10.1016/0022-2836(86)90452-3.
Thastrom A, Bingham LM, Widom J: Nucleosomal locations of dominant DNA sequence motifs for histone-DNA interactions and nucleosome positioning. J Mol Biol. 2004, 338 (4): 695-709. 10.1016/j.jmb.2004.03.032.
Shrader TE, Crothers DM: Artificial nucleosome positioning sequences. Proc Natl Acad Sci USA. 1989, 86 (19): 7418-7422. 10.1073/pnas.86.19.7418.
Ioshikhes IP, Albert I, Zanton SJ, Pugh BF: Nucleosome positions predicted through comparative genomics. Nat Genet. 2006, 38 (10): 1210-1215. 10.1038/ng1878.
Peckham HE, Thurman RE, Fu Y, Stamatoyannopoulos JA, Noble WS, Struhl K, Weng Z: Nucleosome positioning signals in genomic DNA. Genome Res. 2007, 17 (8): 1170-1177. 10.1101/gr.6101007.
Yuan GC, Liu JS: Genomic sequence is highly predictive of local nucleosome depletion. PLoS Comput Biol. 2008, 4 (1): e13-10.1371/journal.pcbi.0040013.
Miele V, Vaillant C, d'Aubenton-Carafa Y, Thermes C, Grange T: DNA physical properties determine nucleosome occupancy from yeast to fly. Nucleic Acids Res. 2008, 36 (11): 3746-3756. 10.1093/nar/gkn262.
Segal E, Fondufe-Mittendorf Y, Chen L, Thastrom A, Field Y, Moore IK, Wang JP, Widom J: A genomic code for nucleosome positioning. Nature. 2006, 442 (7104): 772-778. 10.1038/nature04979.
Fukushima A, Ikemura T, Kinouchi M, Oshima T, Kudo Y, Mori H, Kanaya S: Periodicity in prokaryotic and eukaryotic genomes identified by power spectrum analysis. Gene. 2002, 300 (1-2): 203-211. 10.1016/S0378-1119(02)00850-8.
Mito Y, Henikoff JG, Henikoff S: Histone replacement marks the boundaries of cis-regulatory domains. Science. 2007, 315 (5817): 1408-1411. 10.1126/science.1134004.
Grover D, Mukerji M, Bhatnagar P, Kannan K, Brahmachari SK: Alu repeat analysis in the complete human genome: trends and variations with respect to genomic composition. Bioinformatics. 2004, 20 (6): 813-817. 10.1093/bioinformatics/bth005.
Mighell AJ, Markham AF, Robinson PA: Alu sequences. FEBS Lett. 1997, 417 (1): 1-5. 10.1016/S0014-5793(97)01259-3.
Hamdi HK, Nishio H, Tavis J, Zielinski R, Dugaiczyk A: Alu-mediated phylogenetic novelties in gene regulation and development. J Mol Biol. 2000, 299 (4): 931-939. 10.1006/jmbi.2000.3795.
Polak P, Domany E: Alu elements contain many binding sites for transcription factors and may play a role in regulation of developmental processes. BMC Genomics. 2006, 7: 133-10.1186/1471-2164-7-133.
Englander EW, Howard BH: Nucleosome positioning by human Alu elements in chromatin. J Biol Chem. 1995, 270 (17): 10091-10096. 10.1074/jbc.270.17.10091.
Englander EW, Wolffe AP, Howard BH: Nucleosome interactions with a human Alu element. Transcriptional repression and effects of template methylation. J Biol Chem. 1993, 268 (26): 19565-19573.
Lowary PT, Widom J: New DNA sequence rules for high affinity binding to histone octamer and sequence-directed nucleosome positioning. J Mol Biol. 1998, 276 (1): 19-42. 10.1006/jmbi.1997.1494.
Sharma D, Issac B, Raghava GP, Ramaswamy R: Spectral Repeat Finder (SRF): identification of repetitive sequences using Fourier transformation. Bioinformatics. 2004, 20 (9): 1405-1412. 10.1093/bioinformatics/bth103.
Woodcock CL, Skoultchi AI, Fan Y: Role of linker histone in chromatin structure and function: H1 stoichiometry and nucleosome repeat length. Chromosome Res. 2006, 14 (1): 17-25. 10.1007/s10577-005-1024-3.
Wakaguri H, Yamashita R, Suzuki Y, Sugano S, Nakai K: DBTSS: database of transcription start sites, progress report 2008. Nucleic Acids Res. 2008, D97-101. 36 Database
Lander ES, Linton LM, Birren B, Nusbaum C, Zody MC, Baldwin J, Devon K, Dewar K, Doyle M, FitzHugh W, Funke R, Gage D, Harris K, Heaford A, Howland J, Kann L, Lehoczky J, LeVine R, McEwan P, McKernan K, Meldrim J, Mesirov JP, Miranda C, Morris W, Naylor J, Raymond C, Rosetti M, Santos R, Sheridan A, Sougnez C, Stange-Thomann N, Stojanovic N, Subramanian A, Wyman D, Rogers J, Sulston J, Ainscough R, Beck S, Bentley D, Burton J, Clee C, Carter N, Coulson A, Deadman R, Deloukas P, Dunham A, Dunham I, Durbin R, French L, Grafham D, Gregory S, Hubbard T, Humphray S, Hunt A, Jones M, Lloyd C, McMurray A, Matthews L, Mercer S, Milne S, Mullikin JC, Mungall A, Plumb R, Ross M, Shownkeen R, Sims S, Waterston RH, Wilson RK, Hillier LW, McPherson JD, Marra MA, Mardis ER, Fulton LA, Chinwalla AT, Pepin KH, Gish WR, Chissoe SL, Wendl MC, Delehaunty KD, Miner TL, Delehaunty A, Kramer JB, Cook LL, Fulton RS, Johnson DL, Minx PJ, Clifton SW, Hawkins T, Branscomb E, Predki P, Richardson P, Wenning S, Slezak T, Doggett N, Cheng JF, Olsen A, Lucas S, Elkin C, Uberbacher E, Frazier M, Gibbs RA, Muzny DM, Scherer SE, Bouck JB, Sodergren EJ, Worley KC, Rives CM, Gorrell JH, Metzker ML, Naylor SL, Kucherlapati RS, Nelson DL, Weinstock GM, Sakaki Y, Fujiyama A, Hattori M, Yada T, Toyoda A, Itoh T, Kawagoe C, Watanabe H, Totoki Y, Taylor T, Weissenbach J, Heilig R, Saurin W, Artiguenave F, Brottier P, Bruls T, Pelletier E, Robert C, Wincker P, Smith DR, Doucette-Stamm L, Rubenfield M, Weinstock K, Lee HM, Dubois J, Rosenthal A, Platzer M, Nyakatura G, Taudien S, Rump A, Yang H, Yu J, Wang J, Huang G, Gu J, Hood L, Rowen L, Madan A, Qin S, Davis RW, Federspiel NA, Abola AP, Proctor MJ, Myers RM, Schmutz J, Dickson M, Grimwood J, Cox DR, Olson MV, Kaul R, Shimizu N, Kawasaki K, Minoshima S, Evans GA, Athanasiou M, Schultz R, Roe BA, Chen F, Pan H, Ramser J, Lehrach H, Reinhardt R, McCombie WR, de la Bastide M, Dedhia N, Blocker H, Hornischer K, Nordsiek G, Agarwala R, Aravind L, Bailey JA, Bateman A, Batzoglou S, Birney E, Bork P, Brown DG, Burge CB, Cerutti L, Chen HC, Church D, Clamp M, Copley RR, Doerks T, Eddy SR, Eichler EE, Furey TS, Galagan J, Gilbert JG, Harmon C, Hayashizaki Y, Haussler D, Hermjakob H, Hokamp K, Jang W, Johnson LS, Jones TA, Kasif S, Kaspryzk A, Kennedy S, Kent WJ, Kitts P, Koonin EV, Korf I, Kulp D, Lancet D, Lowe TM, McLysaght A, Mikkelsen T, Moran JV, Mulder N, Pollara VJ, Ponting CP, Schuler G, Schultz J, Slater G, Smit AF, Stupka E, Szustakowski J, Thierry-Mieg D, Thierry-Mieg J, Wagner L, Wallis J, Wheeler R, Williams A, Wolf YI, Wolfe KH, Yang SP, Yeh RF, Collins F, Guyer MS, Peterson J, Felsenfeld A, Wetterstrand KA, Patrinos A, Morgan MJ, de Jong P, Catanese JJ, Osoegawa K, Shizuya H, Choi S, Chen YJ: Initial sequencing and analysis of the human genome. Nature. 2001, 409 (6822): 860-921. 10.1038/35057062.
Xie H, Wang M, Bonaldo Mde F, Smith C, Rajaram V, Goldman S, Tomita T, Soares MB: High-throughput sequence-based epigenomic analysis of Alu repeats in human cerebellum. Nucleic Acids Res. 2009, 37 (13): 4331-4340. 10.1093/nar/gkp393.
Kondo Y, Issa JP: Enrichment for histone H3 lysine 9 methylation at Alu repeats in human cells. J Biol Chem. 2003, 278 (30): 27658-27662. 10.1074/jbc.M304072200.
Luger K, Mader AW, Richmond RK, Sargent DF, Richmond TJ: Crystal structure of the nucleosome core particle at 2.8 A resolution. Nature. 1997, 389 (6648): 251-260. 10.1038/38444.
Gupta S, Dennis J, Thurman RE, Kingston R, Stamatoyannopoulos JA, Noble WS: Predicting human nucleosome occupancy from primary sequence. PLoS Comput Biol. 2008, 4 (8): e1000134-10.1371/journal.pcbi.1000134.
Marino-Ramirez L, Jordan IK, Landsman D: Multiple independent evolutionary solutions to core histone gene regulation. Genome Biol. 2006, 7 (12): R122-10.1186/gb-2006-7-12-r122.
Welch PD: The use of Fast Fourier Transform for the estimation of power spectra: a method based on time averaging over short, modified periodogram. IEEE Transactions on audio and electroacoustics. 1967, AU15 (2): 70-10.1109/TAU.1967.1161901.
Yan M, Lin ZS, Zhang CT: A new fourier transform approach for protein coding measure based on the format of the Z curve. Bioinformatics. 1998, 14 (8): 685-690. 10.1093/bioinformatics/14.8.685.
Tiwari S, Ramachandran S, Bhattacharya A, Bhattacharya S, Ramaswamy R: Prediction of probable genes by Fourier analysis of genomic sequences. Comput Appl Biosci. 1997, 13 (3): 263-270.
Frigo M, Johnson SG: The design and implementation of FFTW3. Proceedings of the Ieee. 2005, 93 (2): 216-231. 10.1109/JPROC.2004.840301.
Langmead B, Trapnell C, Pop M, Salzberg SL: Ultrafast and memory-efficient alignment of short DNA sequences to the human genome. Genome Biol. 2009, 10 (3): R25-10.1186/gb-2009-10-3-r25.
Albert I, Mavrich TN, Tomsho LP, Qi J, Zanton SJ, Schuster SC, Pugh BF: Translational and rotational settings of H2A.Z nucleosomes across the Saccharomyces cerevisiae genome. Nature. 2007, 446 (7135): 572-576. 10.1038/nature05632.
Jiang H, Wong WH: SeqMap: mapping massive amount of oligonucleotides to the genome. Bioinformatics. 2008, 24 (20): 2395-2396. 10.1093/bioinformatics/btn429.
We are grateful to Kengo Kinoshita, Kohji Okamura, Alexis Vandenbon, and other members of the Nakai-Kinoshita Laboratory for a great deal of valuable advice and discussions. Computational time was provided by the Super Computer System, Human Genome Center, Institute of Medical Science, The University of Tokyo. This work was supported in part by Global COE Program (Center of Education and Research for Advanced Genome-Based Medicine), MEXT, Japan.
YT and KN conceived the study and wrote the paper. YT and RY designed the bioinformatics analyses. YS provided the unpublished sequence data of paired-end nucleosomal DNA. YT obtained and analyzed data. All authors read and approved the final manuscript.
Electronic supplementary material
Additional file 1: List of genome sequences used in this study. Sources and versions of genome sequences are listed. (XLS 21 KB)
Additional file 2: Degree of the genome-wide nucleotide periodicity of mono- and di-nucleotide steps from 2 bp to 22 bp. For each mono-/di-nucleotide step, the degree of the nucleotide periodicity within the ranges of 2-22 bp is shown. (PDF 2 MB)
Additional file 3: Degree of the genome-wide nucleotide periodicity of mono- and di-nucleotide steps from 2 bp to 250 bp. For each mono-/di-nucleotide step, the degree of the nucleotide periodicity within the ranges of 2-250 bp is shown. (PDF 1 MB)
Additional file 4: Frequency of mononucleotides within and around Alu elements. Distribution of mononucleotides within and around Alu elements is shown. Red, green, blue and cyan lines represent the frequency of adenine, cytosine, guanine and thymine, respectively. (PDF 622 KB)
Additional file 5: Nucleosome distribution around Alu elements with multi-hit tags considered. Nucleosome distribution around dimeric Alu elements, FLAMs, and FRAMs are shown. In this data, multi-hit tags are included. (PDF 1 MB)
Additional file 6: Distributions of hybridization signals around (A) Alu elements and (B) other repetitive elements. In each cell type (A375, IMR90, MALME, MCF7, MEC, PM or T47D) or in all cells, average hybridization signals around repetitive elements are shown. (PDF 301 KB)
Additional file 7: List of "repName" used for the classification of Alu family. Correspondence between the names of repeats ("repName" in UCSC) and the three Alu types (dimeric Alu elements, FLAMs and FRAMs) are listed. (XLS 18 KB)
Additional file 8: Strategy of detection of sequence tags within ± 150 bp of TSSs. Green arrows represent DNA sequences used as reference sequences. The orientation of the arrow shows the strand. (PDF 31 KB)
About this article
Cite this article
Tanaka, Y., Yamashita, R., Suzuki, Y. et al. Effects of Alu elements on global nucleosome positioning in the human genome. BMC Genomics 11, 309 (2010). https://doi.org/10.1186/1471-2164-11-309
- Repetitive Element
- Nucleosome Position
- Tiling Array
- Nucleosome Core
- Primate Genome