Supplemental methods Biodegradation of dichlorodiphenyltrichloroethanes (DDTs) and hexachlorocyclohexanes (HCHs) with plant and nutrients and their effects on the microbial ecological kinetics Guangdong SUN†*, Xu Zhang†, Qing Hua , Heqing Zhanga, Dayi Zhangb, Guanghe Li†* †. State Key Laboratory of Environmental Simulation and Pollution Control, & School of Environmental Science, Tsinghua University Beijing 100084, China a. China Energy Conservation DADI Environmental Remediation Co., Ltd & State Environmental Protection Engineering Center for Industrial Contaminated Sites and Groundwater Rem ediation, Beijing 100083,China b. Lancaster Environment Centre, Lancaster University, Lancaster, LA1 2YQ, UK * Author for correspondence: Guangdong SUN School of Envrionment, Tsinghua University No.1 Qinghua Park, Beijing 100084, , P. R. China Tel./fax: 86 10 62773232. Email: sungd11@mails.tsinghua.edu.cn Pyrosequencing of 16S rRNA gene amplicon libraries The 16S rDNA was also amplified by PCR for multiplexed pyrosequencing using barcoded primers (Supplementary Table S5). A set of primers was designed by adding a six-nucleotide barcode to the universal forward primer Gray27F and the reverse primer Gray518R (Supplementary Table S3) for amplification of bacteria (V1–V3 regions), 16S rDNA, and target at the hypervariable V1–V3 region. PCR was performed with a thermal cycler (Bio-Rad, Hercules, CA, USA) under the following conditions: initial denaturation at 94°C for 5 min; 26 cycles at 94°C for 30 s, 53°C for 30 s and 72°C for 45 s; and a final extension at 72°C for 6 min. PCR products were detected by 1.2% agarose gel electrophoresis purified using the TaKaRa Agarose Gel DNA Purification Kit (TaKaRa, Dalian, China) and quantified with the NanoDrop device. A mixture of PCR products was prepared by mixing 200 ng purified 16S amplicons from each soil sample and then pyrosequenced on the Roche 454 FLX Titanium platform at the National Human Genome Centre of China, Shanghai, according to the manufacturer’s manual. Quality processing of 16S rRNA gene sequences was performed in Mothur (v.1.28.0) following mainly the 454 SOP that is outlined in [1]. All statistical analyses were conducted in Mothur, JMP 8.0 (SAS Institute, Cary, NC, USA) and R version 2.15.2 (available at http://www.R-project.org). We examined the effects of operational taxonomic unit nucleotide similarity cutoffs on metrics such as diversity and community Bray–Curtis distance at 97%, 95% and 90%. However, as the observed patterns were similar at each cutoff, we used only 97% OTUs (most analyses) and 90% OTUs (correlation network) for final analyses. Singleton sequences that appeared only once in the data set were removed, and each sample was subsampled with the Mothur command “sub.sample” to 1207 reads for 97% OTUs and 1160 reads for 90% OTUs, which was the minimum number of sequences remaining in a single sample. The minimum number of reads per sample was higher for 90% OTUs, because the number of singleton sequences was reduced because of inclusion within larger OTUs. To look at the effect of different treatments on community composition, we used a de-trended correspondence analysis [2]. The de-trended correspondence analysis transformation was performed in R using the “decorana” command in the Vegan package with down-weighting of rare taxa. Significance of the effect of contaminants on community structure was confirmed with a PERMANOVA on community Bray–Curtis values using the “adonis” function in Vegan. The number of OTUs that were shared between contaminant levels was visualized using the Mothur “venn” command. To determine whether bacterial communities were similarly affected by different strategies, we used Mantel tests [3] to compare bacterial community Bray–Curtis dissimilarity matrices from each treatment. In other words, for each treatment, we compared whether the community distances for each possible pairwise combination of samples were related for bacterial communities. We also compared the mean Bray–Curtis dissimilarity value between all bacterial communities within each microcosm and tested for significant differences using one-way ANOVA. Although 454 read abundance is not an exact reflection of the actual taxonomic abundance in situ [4], standardized processing allows the detection of relative shifts between microbial communities. The mean bacterial diversities at each contaminant level were compared using one-way ANOVA. The composition of major bacterial classes was compared between O. violaceus at each contaminant level using UPGMA clustering. Taxonomic abundance data were first normalized using the “decostand” and “vegdist” commands in the Vegan package of R. Rarefaction curves We estimated rarefaction curves for each sample individually as well as compartment-specific rarefaction curves using means at each sampling size for all rarefaction curves of samples belonging to that compartment. Bray–Curtis dendrogram The raw OTU counts were rarefied to 1000 counts per sample employing the function “rarefy” of the R package Vegan. Log2-transformed RA values were used to calculate a Bray–Curtis distance dissimilarity matrix using the function “vegdist” of the R package Vegan. The dissimilarity matrix was used to generate corresponding cluster dendrograms using the function “hclust” of the R package Vegan, specifying the average clustering mode. OCP extraction from soil samples Total OCPs were extracted following the Soxhlet extraction method. All the samples were first spiked with PCB 209 as surrogate standards prior to extraction. The 5.0 g of air-dried soil subsequently underwent Soxhlet extraction for 24 h with hexane/dichloromethane mixture (4:1,v/v) as the extraction solvent (ASE 300; Dionex, Sunnyvale, CA, USA). To improve the extraction efficiency, anhydrous sodium sulfate (5.0 g) and activated copper (1.0 g) were mixed with the soil samples to remove water and sulfur-containing compounds. All extracts were concentrated with a rotary vacuum evaporator system to 1 ml, followed by Florisil solid phase extraction treatment; the cartridge (1.0 g, 6 ml; Supelco, Bellefonte, PA, USA) of which was filled with anhydrous sodium sulfate (2.0 g). The total OCPs were eluted with 40 ml hexane/dichloromethane solvent (9:1, v/v), concentrated to near-dryness by rotary vacuum evaporation, and finally reconstituted in hexane (1 ml) prior to GC analysis. Analytical methods of OCPs OCP analysis was performed using Agilent gas chromatography (7890B) equipped with a Ni-63 electron capture detector and RTX-5 column (30 m × 0.25 mm i.d., film thickness: 0.25 µm). Nitrogen (99.99% purity) was used as the carrier gas at a flow rate of 1.0 ml min–1. The injector and detector temperature were maintained at 260°C and 300°C, respectively. The column temperature was programmed as follows: initial temperature 100°C held for 2 min, increased to 170°C at 25°C min–1, then a ramp at 2°C min–1 to 225°C with the temperature maintained for 2 min, to 290°C at 10°C min–1, and maintained for 8 min. One microliter of the sample was injected in splitless mode. Analytical methods of soil properties Soil samples were air-dried, homogenized and sieved. The particle size distribution was measured by sieving and sedimentation after organic matter destruction (H2O2). The fraction <2 mm was characterized for pH in water suspension (1:2.5, w/v). The organic carbon content was determined by wet combustion. The cation exchange capacity and exchangeable cation was measured by 1 mol l–1 ammonium acetate at pH 7.0. Moisture was determined by placing preweighed contaminated soil samples in an oven at 105°C for 24 h. Total organic carbon was determined according to the Walkley–Black method [5]. Total phosphorus and total nitrogen were analyzed according to standard methods [6]. Soil respiration was measured in triplicate with the Isermeyer method as previously described [7]. Fifty grams of sieved soil (WHC=65%) was transferred into a beaker and placed in an airtight 1.0-l glass jar. CO2 released by basal respiration during 3 days at 25°C was trapped in 25 ml NaOH (0.05 M), which was titrated with HCl (0.05 M) after adding 5 ml BaCl2·12H2O (0.5 M), phenolphthalein as a pH indicator. Nucleic acid extraction and manipulation DNA was extracted in triplicate using an MP FastDNA SPIN Kit according to the manufacturer’s instructions. All extractions were performed immediately following soil sampling to preclude the effects of soil storage on the microbial community. The mass of DNA in each replicate sample was quantified with a Nandrop ND-3300 fluorospectrometer (Nanodrop Technologies, Wilmington, DE, USA) after adding picogreen dsDNA fluorescent indicator dye. DNA and amplified products were purified using Nucleospin Extract II PCR clean-up Gel extraction kit (Macheary-Nagel GmBH). Nucleic acid quantification 16S rRNA and linA-like gene copies were evaluated by a Taqman or SYBR Green based real-time PCR quantification using an iCycler iQ5 themocycler (Bio-Rad), and their primers (Supplementary Table S1) and amplification protocols were specifically described by Suzuki et al., Cebron et al., and Huang et al., respectively [8, 9]. Normalization of gene copies Copy number was normalized by Equation (1) below, where S is the normalized copy number. Cx is the number of targeting gene copies from 1.0 g dry weight soil, and C0 is the number of copies of 16S rRNA extracted from 1.0 g dry weight soil π= πΆπ₯ ⁄πΆ 0 (1) π₯ = {ππππ΄ genes} Reference [1] P.D. Schloss, D. Gevers, S.L. Westcott, Reducing the effects of PCR amplification and sequencing artifacts on 16S rRNA-based studies, PloS one, 6 (2011) e27310. [2] M.O. Hill, H. Gauch Jr, Detrended correspondence analysis: an improved ordination technique, Vegetatio, 42 (1980) 47-58. [3] E. Bonnet, Y. Van de Peer, zt: a software tool for simple and partial Mantel tests, Journal of Statistical software, 7 (2002) 1-12. [4] A.S. Amend, K.A. Seifert, T.D. Bruns, Quantifying microbial communities with 454 pyrosequencing: does read abundance count?, Molecular Ecology, 19 (2010) 5555-5565. [5] E. Bornemisza, M. Constenla, A. Alvarado, E. Ortega, A. Vasquez, Organic carbon determination by the Walkley-Black and dry combustion methods in surface soils and Andept profiles from Costa Rica, Soil Science Society of America Journal, 43 (1979) 78-83. [6] M. USEPA, Methods for chemical analysis of water and wastes, in, Environmental Monitoring and Support Laboratory Cincinnati, OH, USA, 1979. [7] K. Alef, Soil respiration, in: K. Alef, P. Nannipieri (Eds.) Methods in Applied Soil Microbiology and Biochemistry, Academic Press, London, 1995, pp. 214-219. [8] M.T. Suzuki, L.T. Taylor, E.F. DeLong, Quantitative analysis of small-subunit rRNA genes in mixed microbial populations via 5′-nuclease assays, Appl Environ Microbiol, 66 (2000) 4605-4614. [9] A. Cébron, M.-P. Norini, T. Beguiristain, C. Leyval, Real-Time PCR quantification of PAH-ring hydroxylating dioxygenase (PAH-RHDα) genes from Gram positive and Gram negative bacteria in soil and sediment samples, Journal of microbiological methods, 73 (2008) 148-159.