- Research article
- Open Access
Sequencing platform and library preparation choices impact viral metagenomes
© Solonenko et al.; licensee BioMed Central Ltd. 2013
Received: 4 February 2013
Accepted: 2 May 2013
Published: 10 May 2013
Microbes drive the biogeochemistry that fuels the planet. Microbial viruses modulate their hosts directly through mortality and horizontal gene transfer, and indirectly by re-programming host metabolisms during infection. However, our ability to study these virus-host interactions is limited by methods that are low-throughput and heavily reliant upon the subset of organisms that are in culture. One way forward are culture-independent metagenomic approaches, but these novel methods are rarely rigorously tested, especially for studies of environmental viruses, air microbiomes, extreme environment microbiology and other areas with constrained sample amounts. Here we perform replicated experiments to evaluate Roche 454, Illumina HiSeq, and Ion Torrent PGM sequencing and library preparation protocols on virus metagenomes generated from as little as 10pg of DNA.
Using %G + C content to compare metagenomes, we find that (i) metagenomes are highly replicable, (ii) some treatment effects are minimal, e.g., sequencing technology choice has 6-fold less impact than varying input DNA amount, and (iii) when restricted to a limited DNA concentration (<1μg), changing the amount of amplification produces little variation. These trends were also observed when examining the metagenomes for gene function and assembly performance, although the latter more closely aligned to sequencing effort and read length than preparation steps tested. Among Illumina library preparation options, transposon-based libraries diverged from all others and adaptor ligation was a critical step for optimizing sequencing yields.
These data guide researchers in generating systematic, comparative datasets to understand complex ecosystems, and suggest that neither varied amplification nor sequencing platforms will deter such efforts.
Advances in sequencing technologies have revolutionized the life sciences. For example, ecology and evolution can now be examined across the tree of life , and at resolutions ranging from broad analyses (e.g., BGI’s 10,000 Microbial Genomes Project, http://ldl.genomics.cn/page/M-research.jsp) to focused investigation of population structure within particular species . These analyses, however, center on genomes as the unit of interest and represent a “bottom-up approach” to exploring the diversity of life .
Concurrently, metagenomics provides a “top-down approach” for studying complex microbial assemblages in nature . Recent reviews cover next generation sequencing applications [4–6], but rarely acknowledge the factors that generate quantitative data needed for metagenomics. For example, sequence quality evaluated across benchtop systems did not consider library preparation , and recommendations of amplification-free protocols that require >2 μg of DNA to minimize biases  are not meaningful for DNA-limited applications. There are also numerous sequencing platform options, though microbial metagenomes generated across commonly-used sequencing platforms only minimally differ in taxonomic distributions or contig assembly quality .
Some fields, such as viral ecology or microbial ecology of permafrost soils or the atmosphere, are routinely DNA-limited (<1 ng) and thus require optimization and quantitation assessment at each step in the metagenomic sample-to-sequence pipeline . Towards this end, empirical data are now available to guide researchers in concentrating and purifying viruses [11, 12] prior to DNA extraction. Once DNA is extracted, small yields require amplification to obtain enough material for sequencing. While whole genome amplification was an attractive option, it is now documented to result in non-quantitative metagenomes due to both stochastic  and systematic biases . In contrast, linker-amplification-based libraries [15–17] provide a nearly quantitative alternative, even from sub-nanogram amounts of DNA . Together these advances allowed the compilation of the first large-scale, systematically prepared comparative metagenomic dataset for quantitative viral ecology  with new tools and analytical platforms now emerging to handle such datasets [19, 20]. Beyond viral ecology, these studies provide a roadmap for generating quantitative metagenomic datasets from any low (<100 ng) input DNA samples.
Summary statistics for all metagenomic libraries used in analysis
Starting DNA (ng)
Library amplification (# cycles)
Raw reads (millions)
Raw quality +/-SD (PHRED)
Raw length (bp)
Failed QC +/- SD (%)
Biosphere 2 Ocean
Illumina HiSeq 2000
34.2 +/- 0.0
29.9 +/- 0.5
33.8 +/- 0.2
28.3 +/- 0.2 *
Roche 454 GS FLX
32.5 +/- 0.7
408 +/- 11
15.4 +/- 0.4
0.91, 0.90, 0.85
32.8 +/- 0.8
377 +/- 15
31.5 +/- 4.0
Ion Torrent PGM 316 chip
16.3 +/- 0.2
105 +/- 5
40.3 +/- 7.6
Tara Oceans Station 41
Illumina HiSeq 2000
34.2 +/- 0.2
36.2 +/- 0.9
Tara Oceans Station 109
Illumina HiSeq 2000
34.4 +/- 0.5
33.6 +/- 0.6
Experiment 1: The impact of input DNA, amplification, and sequencing platform on metagenomes
Library success varies by sequencing protocol
As expected, the fosmid library and all 6 libraries made from ≥1,000 ng DNA were successful in generating sufficient DNA for sequencing regardless of sequencing platform (Table 1). Additionally, low DNA input libraries for 454 (linker-amplified  to obtain sufficient genetic material) were all successful, with highest read yields per ng of input DNA of any method (Additional file 1: Figure S1).
In contrast, Experiment 1 Illumina libraries constructed from low starting DNA amounts were less successful (Table 1). Specifically, 3 of 6 libraries, one 10ng and both 1ng libraries, failed library construction, even with the addition of carrier DNA and adaptor concentration adjustment to increase ligation efficiencies. Two of the remaining 3 low input DNA libraries, one 10ng and two 100ng, were sequenced, but yielded fewer and more variable numbers of reads and abundant adaptor sequence (see * in Table 1).
%G + C content variation within treatments is minimal
Input DNA amount, decision to amplify impact %G + C content
Hierarchical clustering of sample %G + C distribution correlations shows consistent differences. First, all ≥1,000 ng metagenomes cluster together 100% of the time (Figure 2). Of the treatments tested, input DNA most strongly impacts the resulting metagenomes, with ≥1,000 ng next-generation metagenomes clearly separated from the rest. Among these ≥1,000 ng samples, Illumina metagenomes have higher %G + C than 454 and Ion Torrent metagenomes (see Additional file 1: Figure S2 for example %G + C distribution plots), but differences between sequencing platforms are much less than differences between DNA inputs, with UPGMA branch length distances of 0.02 and 0.16, respectively (Figure 2). While of limited sampling, the largest shift towards higher %G + C sequences (Pearson’s r <0.8) was in the fosmid library relative to the unamplified libraries (Figure 2, Additional file 1: Figure S3).
Among the <1,000ng metagenomes, there are minimal differences between platforms and the only supported relationship, with bootstraps greater than the intra-replicate 94% value, was the clustering of Illumina 100ng samples with Illumina 10 ng samples (Figure 2). This implies that, among amplified metagenomes, the degree of amplification and sequencing platform choice only minimally impact the resulting metagenomes. The fact that these diversely prepared metagenomes were nearly indistinguishable by %G + C distribution metrics (Pearson’s r values >0.99, Figure 2) is promising for comparability of amplified metagenomes across sequencing platforms.
Duplicate reads uncorrelated with any single variable
Duplicates in metagenomes are derived from either naturally occurring duplicates in genomes and communities, or artificial duplicates generated during 454’s emPCR step or at some unknown point in Illumina preparations that is inconsistent across replicate libraries [23, 24].
Here, hierarchical clustering of duplicate frequencies (Figure 2) and raw duplicate distributions, normalized to metagenome size (Additional file 1: Figure S3), suggest a pattern of three duplication groups. The first, composed of unamplified 454 and 10ng Illumina metagenomes, contains intermediate levels of duplication (14.6 to 42.7%) and few high-frequency (>10 fold) duplicate reads (0.06 to 5.1%). The second cluster, composed of most Illumina metagenomes, has an intermediate level of duplication (27.1 to 37.3%), but also an excess of highly duplicated reads (10.4 to 15.6%). The third includes the amplified 454 metagenomes, both Ion Torrent metagenomes, and the poorly amplified 100ng Illumina library, all of which have few duplicate reads (0.9 to 16.6%) and very few high-frequency duplicate reads (0.0005 to 0.9%) (Additional file 1: Figure S4). However, these deep internal nodes lacked support, with bootstraps less than the intra-replicate 90% value, and duplication frequencies do not obviously correlate to any single metagenome category (e.g., technology, amplification, DNA amount, or paired end).
Some duplicate sequences may be real. For example, one 100bp sequence is overrepresented in multiple libraries including 1,000ng Illumina (0.14% of the total reads), Ion Torrent (0.006%), and unamplified 454 (0.36%) libraries. Artificial duplicate frequency correlations (see Online Methods) match overall duplicate frequencies for all treatments except a single 10ng, poorly-amplified, adapter-containing Illumina library (Additional file 1: Figure S5-7), where 40% of the reads were predominantly artificial, high frequency duplicates (Additional file 1: Figure S8 and S9).
Gene function and read assembly parallel %G + C findings
Finally, assembly experiments (see Methods, Figure 3B) revealed that total assembly size positively correlated to the number of reads used in assembly. In turn, the maximum and N50 contig sizes were relatively insensitive to increased read numbers in the larger datasets. This was true for both k-mer and overlap-based assembly algorithms (see Methods).
Experiment 2: The independent effects of input DNA and library amplification on Illumina-sequenced metagenomes
Low input DNA library success improved with optimization
Transposon-based library preparation slightly impacts %G + C
Replication is fundamental to rigorous experimental design , but it is only now becoming financially possible for metagenomic studies [26, 27]. Here we examined replicate metagenomes across varied DNA input amounts, library preparation procedures, and sequencing platforms.
Low input DNA library success depends on adaptor ligation
While all ≥1,000 ng DNA libraries were successful, environmental samples, particularly for viruses, routinely yield <1ng of DNA . Libraries constructed from ≤100 ng DNA were successful using the linker-amplification protocol for 454 , but Illumina libraries failed or were low-quality for Experiment 1, but not Experiment 2. Two separate protocols were used – both optimized for recovery from column purification steps , but employed different template:adaptor ratios in ligation . Specifically, Experiment 1 used 170:1, while Experiment 2 used 22:1 for 10ng starting DNA. Thus low DNA libraries require adjusted adaptor:template ratios during ligation (see Genoscope protocol for guidelines).
Presence of library amplification drives bias
Two amplification reactions are common in metagenomic sample preparations. The first, library amplification, increases input DNA to balance library preparation losses from purification, size selection, and quality titrations . This adaptor-mediated amplification step is used for limiting DNA for 454 (15—25 cycles ), but is routinely employed in Ion Torrent (5 cycles) and Illumina (12—16 cycles) to enrich for correctly ligated adaptors. This step can alter overall library %G + C [15, 17, 30]. The second amplification step is specific to the sequencing technology (e.g., emPCR in 454 or Ion Torrent, bridge amplification in Illumina) and used for improving signal detection. This step should not alter overall library %G + C, but can artificially over-represent sequences [23, 24].
In this study, two libraries received no library amplification: unamplified 454 and fosmid libraries. Fosmids had elevated %G + C, which is ascribed to a cloning bias . Among the remaining libraries, we expected a low %G + C shift due to the adaptor-mediated amplification step, commonly attributed to inhibitory effects of high %G + C DNA secondary structures, either during library amplification  or downstream emPCR . However, these trends were not observed: in Experiment 1, the 454 unamplified and amplified Illumina 1,000 ng libraries correlate well with one another (r-values > 0.99), but poorly (r-values < 0.9) with the amplified (18 cycles) 10ng Illumina libraries. This difference appears to be driven by reduced low %G + C reads relative to the ≥1,000 ng libra ries, which may implicate low input DNA libraries as more sensitive to loss of low %G + C reads either during gel extraction heat steps  or preferential fragmentation through heating . A possible improvement over gel extraction is Sage Science’s Pippin Prep (tested with 65ng of DNA, see Figure 2B in ref. ), which avoids heating. Heat during fragmentation is avoidable with Covaris acoustic shearing. Both techniques also minimize contamination, which is crucial for DNA-limited libraries.
While amplified ≤100 ng metagenomes displayed different %G + C distributions from ≥1,000 ng metagenomes, the amount of amplification only minimally impacts the resulting metagenomes. This was true in Experiment 1, where starting DNA amount and amplification cycling co-varied, as well as Experiment 2, where these parameters were independent. Fragment competition resulting from cycling conditions is thought to select for higher %G + C and shorter fragments, thus linker-mediated amplification protocols employ tight sizing conditions and %G + C optimized PCR conditions . Such careful library construction can produce minimally biased (<1.5-fold %G + C variation) viral metagenomes from sub-nanogram amounts of DNA [10, 15]. The %G + C patterns observed in the current larger-scale study were also paralleled in functional analyses (protein cluster mapping) and assembly performance. This suggests that systematically prepared linker-amplified metagenomes derived from variable input DNA amounts are quantitatively comparable.
Some caution is warranted for high-throughput transposon-based library preparation options like Nextera. Specifically, Experiment 2 revealed that standard libraries prepared from limiting DNA and under varied conditions were relatively invariant, whereas the transposon-based protocol led to divergent %G + C and protein cluster profiles for metagenomes from both stations. While these deviations were statistically significant (90% bootstrap clustering in Figures 4 and 5), they were minor in magnitude relative to other treatment effects observed here. Such a %G + C bias in Nextera library preps is not entirely surprising as previous work demonstrated reduced coverage in both high and low %G + C regions of virus genomes , presumably due to non-random transposition. Evaluation of new transposition methods should be considered if their eventual products require strictly unbiased representation of input DNA.
Finally, while not investigated here, polymerases used in amplification can alter metagenomes. Phi29 polymerase, for example, leads to stochastic and systematic biases that can impact resulting coverage , while some high-fidelity polymerases (e.g., TAKARA) enrich for rare sequences and others (e.g., PfuTurbo) do not [11, 15]. In Experiment 1, the ≥1,000 ng libraries only minimally differed from each other despite the fact that they employ different polymerases across sequencing platforms. These polymerase-specific effects would depend on protocol particulars (e.g., PCR cycler settings and additives) [17, 30] and the underlying %G + C distribution (particularly for <20% or >80% G + C fragments) of the DNA to be amplified. Future work to determine the impact of polymerase choice empirically on metagenomes derived from a wider range of %G + C than those employed here would be informative.
Duplicates vary by input DNA, amplification, technology
Duplicated reads are problematic in quantitative applications as they can be real or artificial [23, 24, 35, 36]. Here, Experiment 1’s true distribution of duplicates is presumably represented by the first cluster (includes unamplified 454 libraries), except the artificial duplicates discussed below. By comparison, metagenomes from the second cluster contained highly duplicated artificial reads that reduced library complexity during amplification. The last cluster, which included amplified 454, as well as one Illumina and two Ion Torrent metagenomes, had low levels of duplication. For the 454 libraries, this could be due to the diversifying effects of the linker amplification process , but it is harder to explain this trend in the Ion Torrent metagenomes or find a process that ties low library amplification in the 100ng Illumina metagenome to lower duplication levels. Artificial duplicates in Illumina libraries were only an issue in the problematic 10ng library, where 40% of the reads were high-frequency, predominantly artificial duplicates. Further study is required to determine mechanisms that generate artificial duplicates in Illumina data.
Sequencing technologies produce comparable output
While the metagenomes here were derived from three very different ocean viral communities, the range of %G + C was not extreme. Given that, sequencing technology is not a major factor impacting ocean viral metagenomes, which is consistent with previous microbial metagenomic studies . However, read length can influence many downstream applications, from assembly efforts to functional identification of genes [37, 38]. Of widely used next-generation technologies, 454 currently has the longest read length of 800bp, with paired-end Illumina capable of 250 + bp . However, emerging nanopore technologies are likely to be truly transformative . Details are not yet public, but these technologies promise longer reads, direct observation of fragment sequences, and minimal library preparation enabling low input DNA applications.
As we strive for systematic and quantitative analyses of complex environments, a thorough understanding of empirically-documented biases in methods is critical. Here we demonstrate that while sequencing platform choice and degree of amplification have little impact on resulting metagenomes, presence of amplification and starting DNA amounts do influence library success and composition. Our findings are critical both for the interpretation of systematic comparisons of DNA-limited community metagenomes, as well as for novel methods of studying virus-host interactions [40–42] that generate small amounts of DNA. Notably, however, high replicability observed here might have been aided by diluting the initial concentrated DNA sample, and potential inhibitors, to obtain ‘low input DNA’ samples. Consideration should be made of the impact of inhibitors on low input DNA samples, particularly when amplification steps are needed for sample preparation.
Given current findings, unamplified libraries are best when DNA is not limiting (>2 ug)  while sequencing platform choice minimally impacts quantitative representation in the resulting metagenomes. When DNA is limiting, as in viral community samples or microbial communities of permafrost soils or air samples, specific recommendations for quantitative metagenomics are as follows. Low input DNA (1—100 ng) libraries can utilize either a linker-amplified protocol  optimized for the appropriate sequencing technology of choice  or, for Illumina sequencing, standard library preparations where adaptor:template ratios are carefully controlled. For samples with ultra-low DNA yields (<1 ng), it is best not to risk failure in standard library preparations and to use instead a sequencing technology optimized linker-amplified protocol. Future research directions include developing a mechanistic understanding of the non-intuitive, but replicable differences in linker-amplified metagenomes, as well as improving understanding of polymerase impacts and developing empirical datasets for a broader range of %G + C samples.
Source DNAs and sample preparation details
Experimental protocol availability
All detailed protocols are listed by name, and are documented and available at http://eebweb.arizona.edu/Faculty/mbsulli/protocols.htm.
Briefly, FeCl-precipitated viral concentrates were obtained from 0.2μm filtered seawater collected from the man-made Biosphere 2 Ocean in December 2010, as well as Stations 41 (Indian Ocean, 14°34.572 N 70°1 E, deep chlorophyll maximum) and 109 (south Pacific Ocean, 1°58.286 N 84°26.772 W, deep chlorophyll maximum) of the Tara Oceans expedition on March 30th, 2010, and May 12th, 2011, respectively. The viral concentrate from the former was purified using both CsCl and DNase, while only DNAse was used for the latter.
DNA Source for B2O metagenomes (Biosphere 2 Ocean)
The B2 Ocean environment is host to a stable microbial community, as measurements of microbial phyletic frequencies are consistent across samples taken a year apart (Additional file 2). FeCl precipitation  was used to concentrate viruses from 1,080L of 0.2 μm filtered seawater, which were then DNase I treated  to remove free DNA, cesium chloride purified to remove microbial contaminants (dsDNA viral band was pulled 1.4—1.52 g/ml ), and further concentrated to 4 mL using an Amicon 30KDa filter. The final yield was 1.26 × 1012 SYBR-stained virus particles. DNA was extracted using the Wizard Prep DNA Purification system (Promega, cat# A7211 and A7181).
DNA Source for TARA metagenomes
20—60L seawater was collected and filtered for two TARA Oceans  stations using the protocol described above. These samples yielded 690 ng (station 41) and 950 ng (station 109) of DNA, using the Wizard Prep DNA Purification system. Starting DNA amounts of 10 and 100 ng were used in Illumina sequencing library construction as described in the Genoscope protocol (Genoscope Illumina protocol).
454 Library Prep (Sullivan lab)
The linker amplification protocol was used to generate amplicon libraries for 454 sequencing, as well as amplification-free libraries, as previously described . Briefly, genomic DNA was Covaris-sheared, unidirectionally ligated to an adaptor, and amplified using adaptor-specific primers using 15 to 25 amplification cycles, depending on the starting DNA amount (a description of the amount of cycling and relationship to input DNA were documented previously ). Following the addition of barcodes, sequencing libraries were ligated to 454-specific adaptors.
Fosmid Library Prep (Hallam lab)
8μg of B2O viral DNA was used in large-insert fosmid library construction using the Epicentre CopyControl Fosmid Library Production Kit (CCFOS110) as previously described . A total of 17 384-well plates of clones were picked, and 384 fosmids were sequenced bi-directionally with Sanger sequencing.
Ion Torrent Library Prep (University of Arizona Genomics Core)
2μg of B2O viral DNA was used for sequencing library preparation following the Ion Fragment Library Kit User Guide (Rev July 2011), loaded onto beads, emPCR-ed, then sequenced using the 316 chip on the Ion Torrent PGM.
Illumina Library Prep for B2O metagenomes (Emory Genomics Core)
DNA samples were Covaris-sheared and size-selected to 300—600bp using SPRI Size Selection chemistry, enrichment amplified using Phusion DNA polymerase according to starting amount of DNA (14—18 cycles), and paired end sequenced. Two libraries starting with 1ng of DNA failed to amplify to sufficient amounts, even with the use of a carrier DNA protocol (Emory carrier DNA protocol). One 10 ng library experienced the same problem, and was not sequenced. The libraries were multiplexed on two sequencing lanes, with one replicate of each starting amount library present together on each lane.
Illumina Library Prep for TARA metagenomes (Genoscope)
DNA samples were Covaris-sheared and size selected to 160—180bp, amplified according to starting amount of DNA (9—15 cycles) and paired-end sequenced. Several modifications of the standard Illumina protocol  were introduced in order to minimize losses of ultra-low DNA amounts. The low-fragment-size shearing settings, coupled with Ampure beads to remove very short fragments, ensured the recovery of appropriately sized fragments without the need for gel sizing. The Pfx Platinum polymerase was used to increase amplification efficiency and thus decrease the number of total library amplification cycles. During ligation, proper adaptor ratios were chosen to correspond to 2—3 fold more adaptor ends than fragment ends in the working ligation reaction (Genoscope Illumina protocol). Transposon-based Nextera libraries were prepared per manufacturer’s instructions using the Illumina compatible Nextera DNA Sample Prep Kit (Epicentre Biotechnologies, cat#GA09115).
All custom scripts are listed by name and available at http://code.google.com/p/tmpl/.
All metagenomic sequences are publically available through the CAMERA portal at http://camera.calit2.net/ [CAMERA: CAM_P_00001027]. 454 and Ion Torrent data, provided by UAGC, were delivered in .sff format and converted for downstream processing to FASTA and QUAL formats using sffinfo (roche454 v2.6) and then to FASTQ format using BioPerl 1.6.1. B2 Ocean Illumina data, by Emory Genomics Core, and TARA Oceans Illumina data, by Genoscope, were provided in FASTQ format. Each library was examined for raw quality using FastQC (v0.9, downloaded Aug 2012 from http://www.bioinformatics.babraham.ac.uk/projects/fastqc/) and Fastx_Toolkit (v0.0.13 downloaded Feb 2010 from http://hannonlab.cshl.edu/fastx_toolkit/). The FastQC report was the source of duplication data used in the figures. Adapter sequences were detected in two metagenomes (I1A18N10 and I1A14N100) through the overrepresented sequences functionality of FastQC. The fastx_toolkit utility ‘fastx_clipper’ was used with the –C option to remove all reads matching the above adapter motif from the forward paired end reads, removing approximately 40% of the reads that passed QC in each of these libraries.
Next, procedures for quality control were established to remove suspect sequence data, either by filtering whole reads or trimming reads in accordance with known sequencing technology artifacts. For 454 and Ion Torrent data, whole-read filtering was used, as is common for metagenomics [11, 15, 45, 46] (Additional file 1: Figure S10). In contrast, because Illumina errors are localized to particular parts of a read [47, 48], these data were trimmed using a threshold predicted quality score to remove suspect regions of the read at both the 3’ and 5’ ends using DynamicTrim.pl, part of the SolexaQA package  (Additional file 1: Figure S11). After QC steps, 69—85% of the 454 reads remained, compared to 60% for Ion Torrent and 63—74% for Illumina (Table 1). The fastx_toolkit software package was also used to remove Illumina reads under 50bp, while the 454 and Ion Torrent reads were cleaned using a custom pipeline . This processing ensured that the data analyzed would be analogous to that used for metagenomic inference. FastQC and Fastx_Toolkit were used to check the QC process of each metagenome.
%G + C analytics
The mean read %G + C was chosen as the focus of our analysis, rather than the %G + C of sequence subsets of a read or the larger genome regions from which the read fragment originated, since mean fragment %G + C the best predictor of GC bias . QC-ed reads were processed using the BioPerl 1.6.1 script bp_gc_calc.pl to obtain average %G + C values for each read. Given the large read length differences across these libraries (90bp to 350bp), only the first 50bp of each read are used in all %G + C distribution analyses to match the shortest QC-ed Illumina data, while normalizing for read length. Reads were truncated to 50bp using fastx_toolkit and processed with bp_gc_calc.pl. Phage metagenomic reads were cut into non-overlapping 50bp fragments using a bash script and also processed with bp_gc_calc.pl.
Statistical analysis and figures
R 2.14.1 (http://www.R-project.org/) was used to run a custom script, 0.02gc.R, which calculated frequencies of reads in 2% G + C bins for each metagenome. Pearsons’s r pairwise correlation values were calculated using the cov() function, and heatmap figures were generated using the heatmap.2() function found in the gplots library (http://CRAN.R-project.org/package=gplots). Lastly, bootstrapped UPGMA clustering values for each node were obtained using the pvclust() function in the pvclust library (http://CRAN.R-project.org/package=pvclust), with pairwise distances calculated from Pearson’s correlation values and hierarchical clustering done using the “average” method.
Duplication levels were assessed in raw reads by counting the occurrence of duplicates only in the starting 50bp of each read using the FastQC duplication level utility output, normalized to total metagenome size to reflect relative frequencies. Artificial duplicates were defined as those with identical starts and >95% identity throughout the read, and were detected using CD-HIT-454  and CD-HIT-DUP  with default parameters.
Protein cluster analyses
Functional differences within and between metagenomes were assessed in Experiment 1 by mapping metagenomic reads to the Pacific Ocean Virome database . The hit frequencies of the 1,500 protein clusters that were most abundant across all metagenomes were then used to obtain pairwise correlation values. A range of 3—7% of the metagenomic reads mapped to these POV PCs, while the ‘top 1,500 PCs’ subsample represented >99% of the data that mapped. Because the Experiment 1 dataset represented a large diversity of read lengths, greatly impacting inference capacity , the dataset was normalized to assess sequencing platform biases rather than read length impacts as follows: (i) the longer Ion Torrent and 454 reads were trimmed to 100bp, and (ii) only reads ≥100 bp were used from Illumina data.
The short reads derived from Illumina and Ion Torrent data were assembled using Velvet v 1.2.03  using default parameters across a range of kmer sizes (23, 27, 31bp), but only 31-mer data are reported as kmer size did not impact assemblies. The longer 454 reads were assembled using GS De Novo Assembler v2.6 (http://my454.com/products/analysis-software/index.asp) with default parameters.
We thank B. Poulos, N. Solonenko, A. Gregory, and C. Decker for technical assistance, as well as TMPL members and two anonymous reviewers for comments on the manuscript. Funding for this particular study was provided by BIO5, Biosphere 2 and the Gordon and Betty Moore Foundation to MBS. We thank the coordinators and members of the Tara Oceans consortium (http://www.embl.de/tara_oceans/start/) for organizing sampling and data analysis. We thank the commitment of the following people and sponsors who made this singular expedition possible: CNRS, EMBL, Genoscope/CEA, VIB, Stazione Zoologica Anton Dohrn, UNIMIB, ANR (projects POSEIDON/ANR-09-BLAN-0348, BIOMARKS/ANR-08-BDVA-003, PROMETHEUS/ANR-09-GENM-031, and TARA-GIRUS/ANR-09-PCS-GENM-218), EU FP7 (MicroB3/No.287589), FWO, BIO5, Biosphere 2, agne`s b., the Veolia Environment Foundation, Region Bretagne, World Courier, Illumina, Cap L’Orient, the EDF Foundation EDF Diversiterre, FRB, the Prince Albert II de Monaco Foundation, Etienne Bourgois, the Tara schooner and its captain and crew. Tara Oceans would not exist without continuous support from 23 institutes (http://oceans.taraexpeditions.org). This article is contribution number 0005 of the Tara Oceans Expedition 2009–2012.
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