- Open Access
High-throughput profiling of point mutations across the HIV-1 genome
© Al-Mawsawi et al.; licensee BioMed Central. 2014
Received: 8 September 2014
Accepted: 4 December 2014
Published: 19 December 2014
The HIV-1 pandemic is not the result of a static pathogen but a large genetically diverse and dynamic viral population. The virus is characterized by a highly mutable genome rendering efforts to design a universal vaccine a significant challenge and drives the emergence of drug resistant variants upon antiviral pressure. Gaining a comprehensive understanding of the mutational tolerance of each HIV-1 genomic position is therefore of critical importance.
Here we combine high-density mutagenesis with the power of next-generation sequencing to gauge the replication capacity and therefore mutational tolerability of single point mutations across the entire HIV-1 genome. We were able to achieve the evaluation of point mutational effects on viral replicative capacity for 5,553 individual HIV-1 nucleotide positions – representing 57% of the viral genome. Replicative capacity was assessed at 3,943 nucleotide positions for a single alternate base change, 1,459 nucleotide positions for two alternate base changes, and 151 nucleotide positions for all three possible alternate base changes. This resulted in the study of how a total of 7,314 individual point mutations impact HIV-1 replication on a single experimental platform. We further utilize the dataset for a focused structural analysis on a capsid inhibitor binding pocket.
The approach presented here can be applied to any pathogen that can be genetically manipulated in a laboratory setting. Furthermore, the methodology can be utilized under externally applied selection conditions, such as drug or immune pressure, to identify genetic elements that contribute to drug or host interactions, and therefore mutational routes of pathogen resistance and escape.
Currently ~35 million people are living with human immunodeficiency virus-1 (HIV-1) infection, the pathogen responsible for acquired immunodeficiency syndrome (AIDS), with tens of millions having died of AIDS-related causes worldwide since the pandemic began (UNAIDS. GAP Report; 2013). The virus rapidly evolves due to the high error rate of the viral reverse transcriptase (RT) enzyme at 3.4 × 10−5 mutations per site per generation coupled with a rapid generation output rate of ~1 × 1010 virions per patient per day -, and the propensity of RT to mediate RNA recombination via template switching during genomic reverse transcription at ~10 times per replication cycle ,. This genetic plasticity renders many vaccine candidates effective at neutralizing only a subspecies of the virus within the patient, and drives the ongoing challenge of antiretroviral resistance in HIV-1 therapy. It is therefore of paramount importance that we gain an understanding of the mutational tolerance of the HIV-1 genome in exquisite detail to effectively design strategies to prevent, treat, and ultimately diminish the damage to human health. Here we provide a replication capacity (RC) analysis of 57% of the HIV-1 genome for single point mutations using a high-throughput genetic approach that combines high-density mutagenesis with the power of next-generation sequencing (NGS) we term quantitative high resolution genetics (qHRG). The RC dataset can be further used to assist in HIV-1 vaccine design, identification of nucleotide-level cis functionalities, and structural annotation to aid in drug development - an example of which, using the viral capsid protein, is given. qHRG can be applied to other viral pathogens and under any applied selection condition that may be relevant to viral pathogenesis.
Point mutation library construction
Mutant library selection and next-generation sequencing
Each mutant plasmid library was reconstituted into virus, and passaged in CEM T-lymphocytes in an iterative and parallel fashion for four rounds. For each passage, supernatant was collected, titered, and added to ~20 million cells at a MOI of 0.01 to initiate the next selection round. Virion RNA was isolated after each passage, reversed transcribed, and quantified using qPCR. Transcript levels for each input plasmid and all selection rounds were high enough to maintain the full complexity of each starting library, and we therefore could accurately quantify relative frequencies of each variant following each round. Initial deep sequencing experiments on single amplicon stretches within the gag, pol, and env genes of the viral genome for each passage round indicated RC selection was largely complete by passage round 2 (R2). Furthermore, mutant complexity is largely retained from DNA plasmid to reconstituted viral particles during the transfection step, with a correlation of 85-95% across different libraries. We therefore focused on the input plasmid libraries and R2 egressed viral libraries for RC analysis across the entire HIV-1 genome (qPCR transcript levels for each shown in Additional file 2A). The complete cell culture passage scheme is provided in Additional file 3. We conceptually designed a two-step PCR strategy to prepare isolated virion cDNA that is specific for the NGS Illumina platform (Figure 1B). Following HIV-1 cDNA generation, the first PCR step utilizes HIV-1 library specific primers to generate short (~188 bp) amplicons with each containing a unique nucleotide sequence tag and constant regions at each terminus corresponding to the adaptor regions required for the Illumina sequencing platform. The generation of each PCR product is confirmed by electrophoresis, and library-specific amplicons are pooled and subjected to a single sub-saturation PCR affixing the remaining Illumina adaptor region required for NGS. The final products were then sequenced on an Illumina HiSeq2000 machine using paired-end 2 × 100 read parameters. The amplicon-based technique ensures uniform representation of the entire genome as compared to traditional shearing methods which often result in over-representation of DNA fragment ends. The approach also affords unique nucleotide sequence tags and the adapter region specific for the Illumina platform in the primer design, and includes an error-correction step to clearly distinguish true mutation versus NGS instrument error from the output sequencing reads. Our strategy ensures an accurate count for each discrete amplicon present in the selection pool, which through clustering of unique sequence tags present on each amplicon, quickly identifies sequencing errors, a procedure conceptually similar to a method previously described . However, our strict limitation on redundancy ensures sequence space is maximized to achieve error correction without losing sequencing depth on the finite Illumina platform. Another key for confident quantification of relative frequencies in this strategy is to have a diverse enough combination of unique sequence tags to cover all individual WT and mutant species present in the selection pool (see Methods).
Calculation of point mutation replication capacity
RC index = (occurrence frequency in R2)/(occurrence frequency in plasmid library).
Validation of missense mutation replication capacity
qHRG missense mutation experimental validation
HIV-1 genomic region
DNA coverage a
qPCR value b
Application of missense mutation replication capacity profile
Structural annotation of qHRG RC data can provide valuable insight to help explain functionalities of viral proteins for a multitude of aspects relevant to viral replication and disease progression. Protein RC views in three-dimensional space allow for the detection of structurally adjacent positions with similar RC costs upon substitution not readily apparent if focusing on a specific protein region on the primary sequence. This can aid in assessing the genetic barriers of resistance in existing drug binding sites to guide inhibitor optimization, and can provide for the discovery of altogether novel binding pockets, where regions of low substitution tolerability can be used for therapeutic development in combination with computational techniques.
In this study we used our high-throughput genetic platform to assess the impact of point mutations on viral RC in an X4 laboratory HIV-1 strain in T-lymphocyte cell culture. The RC of mutations at each nucleotide position strictly reflects this experimental condition. Interestingly, mutations that resulted in a RC greater than the WT pNL4-3 strain (RC index >1) were very rare and amounted to only 1.9% of the complete dataset (140 out of 7,314 total mutations) providing indication that pNL4-3 is already well adapted to cell culture growth and optimization resulting from substitutions, at least resulting from one mutational step away from WT, is not a common occurrence. Our methodology could be utilized to define nucleotide positions that confer a RC advantage under other selection conditions such as HLA escape or drug resistance, or other genetic backbones such as a M-tropic CCR5 utilizing strain. Employing qHRG under different HIV-1 relevant selection conditions with multiple genotypes and compiling the data will provide a more comprehensive map of the genetics of HIV-1 pathology. Moreover our RC data may overlap with sequence conservation information that is readily available from patient derived HIV-1 sequence databases, but conservation of a particular nucleotide position does not strictly equate to a high RC for that viral position ,, but a direct RC advantage of a select ancestral strain in that particular patient environment. qHRG provides a complementary, direct, and functionally-based approach to impartially identify amino acid residues that are critical for viral replication in a defined cellular environment. To complement data collected from naturally occurring variations in clinical samples, our approach can be applied to study the dynamics of viral mutant populations in different growth conditions with precise control of experimental conditions to directly ascertain the mechanistic interplay between virus and host.
In the course of applying our genetic profiling approach on the complete HIV-1 genome, we have identified a number of improvements that can be incorporated in the future usage of our methodology. Since multiple mutations were introduced for individual clones in the mutant libraries in this study, a systematic mutational additive effect may be present during the quantification of individual mutation RC. It is possible that our mutation rate (~5 mutations per kb) resulted in a ‘dragging-down’ effect for neutral mutations especially in enzymatic protein coding regions, where subsequent deleterious mutations present on the genome with the mutation of interest created an average RC value to be lower than expected. The obtainment of larger mutant library pools, which would afford a higher coverage at each nucleotide position, would considerably improve the RC data at silent mutational positions exhibiting a neutral phenotype. Longer sequencing reads, which are becoming increasingly available on multiple NGS platforms, would also address epistatic effects. Additionally, this problem can be resolved by lowering the number of mutation rate to 1–2 per clone, which becomes more feasible and affordable with the increasing capacity of NGS technology. In addition, the high mutation rate within the HIV-1 replication cycle may increase the noise of RC profiling and obscure the identification of a lethal mutation. Mutational assessment could be further refined by increasing the input occurrence frequency of individual point mutations by performing random mutagenesis on a shorter fragment. A more dramatic drop of occurrence frequency will be detected if a lethal mutation has a higher occurrence in the input mutant library. In other words, the calculated RC value will be lower for a lethal mutation that has a higher occurrence in the input mutant library. We anticipate the above technical improvements would enrich the quality of the RC profiling data.
This study represents the first application of our qHRG method to an entire viral genome – namely HIV-1. However, our platform will be useful for any virus that can be genetically manipulated in a laboratory setting. We recently demonstrated the power of our sequencing approach for viral drug development using the NS5A protein of hepatitis C (HCV) under the inhibitory pressure of Daclatasvir to help predict clinical outcomes if development continued to therapeutic use . For influenza A, we have profiled RC of the hemagglutinin gene at single-nucleotide resolution , profiled for mutations affecting type 1 interferon sensitivity in the NS segment , and uncovered compensatory mutations to Tamiflu in the neuraminidase gene . As demonstrated in our HCV study, we show how the comprehensiveness of qHRG can be increased by applying saturation mutagenesis for library construction, which enables the interrogation of every codon for all possible amino acid substitutions, and removes the experimental limitation of only examining substitutions that can be obtained by one mutational step away from WT. We have also demonstrated the application of our amplicon-based PCR approach for Illumina NGS to clinical HIV-1 quasi-species populations in acute infection  and achieved a higher sensitivity in identifying rare quasi-species variants as compared to published approaches using other NGS platforms. A number of groups have also been utilizing high-resolution mutational scanning combined with NGS that targets proteins or protein domains to gain insight into protein function and evolutionary mutational tolerance -.
We have provided a RC map of the HIV-1 genome using a genetic platform that combines high-density mutagenesis with NGS. The utility of such a comprehensive RC dataset is extensive. Examples include (i) determining regions less tolerable to mutation to aid in vaccine or therapeutic development, (ii) identification of nucleotide sequence changes that result in a lethal replication phenotype, but encode silent substitutions at the amino acid level – suggesting function at the nucleic acid level, ie., RNA secondary structure, DNA-protein recognition signals, or small RNAs, and (iii) structural annotation of essential amino acids on existing three-dimensional structures to provide insight into structure-function relationships. Here, the power of our qHRG platform is the ability to sensitively quantify the RC of individual viral variants in a large and diverse population of mutants for involvement in a replicative pathogenic process within a well-defined biological environment on a single experimental platform.
Viral mutant library preparation
To generate the HIV-1 mutant library we designed a PCR strategy utilizing the HIV-1 proviral DNA plasmid pNL4-3 as template and the error-prone polymerase Mutazyme II (Strategene) to generate the point mutations during PCR amplification. The HIV-1 genome of the molecular clone pNL4-3 was divided into 7 segments ranging from ~1.3 to 2.3 Kb. Fragment start and end sites were selected based on the location of unique enzyme digest restriction sites within the plasmid. We further designed primer sets overlapping each distinct restriction site for error-prone PCR and validated the primer pairs for efficient PCR amplification. All primers used in this study are given in Additional file 8. Error-prone PCR was conducted using the GeneMorph II Random Mutagenesis Kit (Stratagene) and a starting target mutagenized fragment region amount of either 0.5 ng (fragment 1, 2, and 6) or 5 ng (fragment 3, 4, 5, and 7). All error-prone PCR reactions contained an initial melt step at 95°C for 2 min and a final extension step at 72°C for 10 min, followed by a final hold at 4°C. Repetitive error-prone PCR cycle parameters were fragment specific according to optimized primer annealing temperatures, extension times due to fragment length, and cycle numbers to obtain a target mutation rate of as close to ~5 mutations per kilobase as possible. For each fragment: Frag1: 95°C 30 sec, 63°C 30 sec, 72°C 2 min 15 sec, 40 cycles; Frag2: 95°C 30 sec, 55°C 30 sec, 72°C 1 min 30 sec, 30 cycles; Frag3: 95°C 30 sec, 63°C 30 sec, 72°C 1 min 30 sec, 30 cycles; Frag4: 95°C 30 sec, 63°C 30 sec, 72°C 2 min 15 sec, 40 cycles; Frag5: 95°C 30 sec, 55°C 30 sec, 72°C 1 min 30 sec, 30 cycles; Frag6: 95°C 30 sec, 56°C 30 sec, 72°C 1 min 30 sec, 30 cycles; Frag7: 95°C 30 sec, 65°C 30 sec, 72°C 1 min 30 sec, 40 cycles. To eliminate WT background contamination we constructed seven new pNL4-3 vectors, where we swapped each ~1.3-2.3 kb WT fragment with a small 15 nucleotide fragment that contained the corresponding restriction sites at either end and a new unique MluI site within the fragment as a “kill-site” not originally present in the pNL4-3 vector. The seven vectors were strictly used to sub-clone each mutant fragment PCR product back into pNL4-3 resulting in a full length proviral genome, and enabled us to use PCR clean-up columns to remove the 15 base pair insert after vector digestion resulting in very clean ligations. This cloning strategy further ensured no WT background species will contaminate our libraries by (1) using the MluI kill-site to further remove background, and (2) guaranteed that if background was present after ligation the viral genomes would be missing greater than a kilobase of genome and result in non-viable viral particles. Mutagenized PCR fragments were ligated into each corresponding digested cloning vector using T4 DNA ligase (Invitrogen), transformed into chemically competent DH5α (fragments 2 and 3) or electroporated using a Gene Pulser II (BioRad) into MegaX DH10B T1R (Invitrogen) E.Coli according to manufacturer’s instructions and plated on four 143 cm2 ampicillin agar plates. For each fragment, colonies were counted, scraped and pooled into ~25 mL LB and the plasmid was midi-prepped (Invitrogen). The mutation rate per fragment and coverage for each fragment nucleotide position base change are as follows: Frag1: 4.5 mutations per 711 base pair region; 64,781 colonies obtained resulting in 134-fold coverage for all mutations at each fragment position. Frag2: 6 mutations per ~1300 base pair region; 49,968 colonies obtained resulting in 77-fold coverage for all mutations at each fragment position. Frag3: 10 mutations per ~1500 base pair region; 39,240 colonies obtained resulting in 87-fold coverage for all mutations at each fragment position. Frag4: 14 mutations per ~2300 base pair region; 54,605 colonies obtained resulting in 110-fold coverage for all mutations at each fragment position. Frag5: 8.5 mutations per ~1500 base pair region; 62,598 colonies obtained resulting in 118-fold coverage for all mutations at each fragment position. Frag6: 6 mutations per ~1600 base pair region; 79,750 colonies obtained resulting in 99.5-fold coverage for all mutations at each fragment position. Frag7: 4 mutations per 832 base pair region; 127,406 colonies obtained resulting in 204-fold coverage for all mutations at each fragment position.
Passage of HIV-1 mutant libraries in CEM T-lymphocyte cell culture
Each HIV-1 mutant plasmid library was separately transfected in 293T cells for viral propagation. Cell culture supernatant after transfection and after each CEM T-cell passage was measured for p24 levels using the CFAR Virology Core Facility at UCLA, filtered with a 0.22 μM MCE filter (Fisher Scientific) and subsequently added to 2 × 107 cells (cell number calculated to maintain library complexities) at a MOI of 0.01 with 2 μg/mL polybrene to initiate the next selection round. This process was conducted in an iterative and parallel fashion for four rounds to select out viral species containing mutations that deleteriously effect replication capacity. Supernatant p24 levels were used to estimate MOI. p24 provides a measurement of viral particle concentration regardless of potential infectivity, often providing an inflated value for MOI calculation. We compared the p24 derived MOI calculation with a tissue culture infectious dose (TCID) limited dilution assay and determined the discrepancy between final values was generally less than one log (p24 > TCID). For all library selection rounds we maintained a low p24 calculated MOI (0.01) to minimize possible trans-complementation between viral variants in the same infected cell. Although this MOI can be considered ≤0.01, further reducing possible trans-complementation, it was not viewed as an experimental obstruction as cell numbers for each selection round were maintained in surplus to assure coverage of the starting library complexities. For each passage, at 24 hours post infection, cells were centrifuged, PBS washed, and re-suspended in fresh RPMI media to remove unadsorbed virus. HIV-1 induced cytopathic effects were visually monitored, and each selection round was typically terminated ~7-10 days post infection. Virion RNA was isolated from cell culture supernatants using QIAamp Viral RNA kit (Qiagen) and reverse transcribed to cDNA using Superscript III Reverse Transcriptase (Invitrogen) using random hexamers. cDNA was then quantified using sybr green qPCR with known concentrations of linearized pNL4-3 plasmid as standards and primers specific to the env gp41 region of the viral genome validated for efficiency previously (m = −3.3, R2 = 0.9985), on a DNA engine Opticon 2 real-time cycler (BioRad), using cycle parameters 95°C 3 min, 95°C 20 sec, 56°C 20 sec, 72°C 45 sec, 40 cycles, 72°C for 10 min, and a final hold at 4°C, and data was further used to calculate transcript count.
Next-generation sequencing of virus mutants
We conceptually designed a two-step PCR strategy to prepare isolated viral RNA (cDNA) after each selection round that is specific for the NGS Illumina HiSeq 2000 platform. Virion cDNA was used as template to amplify amplicons that are ~188 nts using HIV-1 specific primer pairs. The primer space between library fragments 1–7 was constant and therefore not covered in mutagenic selection: primer space 1–2: nucleotides 705–724, 2–3: nucleotides 1995–2022, 3–4: nucleotides 3477–3500, 4–5: 5733–5760, 5–6: 7244–7268, and 6–7: 8878–8898. Each primer pair (69 staggered pairs for genome covered – nucleotides 147–9606, LTR regions 1–146 and 9607–9709 of 5’ and 3’ ends of genome not sequenced) contains a unique nucleotide tag among them consisting of 10 random nucleotides to identify the specific amplicon fragment combined with either two keto bases “K” (T or G) or two amino bases “M” (C or A) to identify the DNA input or R2, respectively. The total number of possible unique nucleotide tag sequences is 4,194,304, ensuring that each individual amplicon in the pool has a unique identifying sequence, and importantly was diverse enough to cover both WT and mutant species. The primer pairs also contain part of the 5’ and 3’ Illumina adapter regions required for sequencing at their termini. For all HIV-1 specific amplicon PCR reactions of step one we used high-fidelity KOD DNA polymerase (EMD Millipore) with the cycle parameters 95°C 2 min, 95°C 20 sec, 56°C 20 sec, 68°C 45 sec, 40 cycles, 68°C for 10 min, and a final hold at 4°C, with the exception of fragment 1 amplicon 5, and fragment 2 amplicon 1, which utilized the annealing temperature of 66°C. Once HIV-1 amplicon fragments were amplified from each round, an aliquot (~5 μL) was electrophoresed on a 3% agarose gel to confirm PCR product amplification. Aliquots (~5 μL) of each HIV-1 amplicon product required for one NGS Illumina HiSeq 2000 sequencing lane were pooled and spun through a PureLink PCR purification column (Invitrogen). We have overcome an inherent NGS error-correction issue by ensuring ten copies of each amplicon is sequenced in order to distinguish mutation versus sequencing error. Based on manufacture information at the time we conducted our experiment the error rate for the HiSeq 2000 NGS platform ranged from 0.1-1%, whereas the typical output per lane of the instrument was ≥150 million filtered reads. For all our calculations, we conservatively estimated the filtered read output per lane at 120 million reads to ensure we obtained sufficient coverage per amplicon. In previous optimization trial experiments using the instrument we directly observed the error rate as low as 0.1%, a rate that still poses a significant challenge to accurately calling true mutations versus instrument error in such a large diverse mutant population. To effectively identify instrument errors, we precisely quantified the number of pooled amplicon molecules from PCR step one, and subsequently decreased the amplicon number to 12 million molecules (typically a dilution of ~12,500X) before it is used as template for the Illumina specific PCR in step two ensuring that a median of 10 copies of each amplicon are present after a sub-saturation (18–20 cycles) PCR.
A cluster containing only three or less reads were filtered removed. In addition, only a mismatch that had an occurrence of >95% within a cluster was called as a true mutation. This criteria provided a high statistical confidence with a p-value ≤ 10−9 (binomial exact test) for individual mutation calling. One potential pitfall was that it is possible to have two or more WT copies carrying the same unique nucleotide tag as input for the second step PCR. This would result in an underestimation of WT copy number. Nonetheless, the input copy number for the second PCR was estimated to be ~85,000, which is 50-fold lower than the unique nucleotide tag complexity. The possibility of having any two different molecules carrying the exactly same unique nucleotide tag would be ~0.02% (approximated by Poisson distribution, λ = 85,000/4,194,304). Therefore, the underestimation of WT copy number is very minimal.
Using this approach the sensitivity to detect rare variants was dependent on amplicon coverage, and therefore varied by amplicon and selection round (Additional file 4). For sensitivity, we typically achieved the ability to detect mutants as rare as 0.001% in the viral population after error correction. With the exception of amplicon F1-A5 (nucleotides 568–704), where coverage was consistently low for both input and R2 (sensitivity range of 0.009-0.01%), and amplicon F1-A4 (nucleotides 417–567), where coverage was low in R2 (sensitivity of 0.06%), our sensitivity range to detect rare mutations was 0.0004-0.001% and 0.0008-0.009%, for DNA input and R2, respectively.
Another important aspect to consider in planning our high-scale mutation experiment in achieving a sensitivity after NGS sequencing is to determine true mutation frequency changes above what may be imparted by the cDNA synthesis error rate at 3.4 × 10−5. We determined the number of library mutations achieving an input DNA frequency (mutation coverage/amplicon coverage) greater than the reported cDNA synthesis error rate. As can be seen in Additional file 9, frequency of engineered mutations in our library predominately achieves a log scale fold-increase above the cDNA synthesis error rate.
The purified PCR step one amplicon pool was measured via nanodrop, exact DNA molecules calculated, and diluted appropriately to 12 million molecules per lane for error-correction (~12,500X). A single sub-saturation PCR to add on the final regions of the Illumina adapter region was then conducted on the diluted PCR product using high-fidelity KOD DNA polymerase (EMD Millipore) with the cycle parameters 95°C 2 min, 95°C 20 sec, 62°C 20 sec, 68°C 45 sec, 20 cycles, 68°C for 10 min, and a final hold at 4°C. Product from the second PCR was spun through a PureLink PCR purification column (Invitrogen), eluted in dH2O, and a 15 μL aliquot at ~8 ng/μL was provided to the DNA Microarray Core Facility at UCLA, where the concentration was confirmed by Qubit, the size and quality confirmed using a Bioanalyzer (Agilent Technologies), and subsequently sequenced on an Illumina HiSeq2000 machine using paired-end 2 × 100 read parameters. Raw sequencing data were deposited to the NCBI Sequence Read Archive (SRA) under accession code BioProject PRJNA259391.
Recently, similar NGS error-correction approaches of ensuring redundancy of unique identifying sequences was independently reported as a means to identify rare cellular mutations and variants within a single gene focused pool ,. The study by Jabara et al. used an 8-mer degenerate nucleotide sequence at the cDNA synthesis step to uniquely identify patient derived HIV-1 PR variants . Unique sequence tagging at the cDNA synthesis step would prove highly beneficial as cDNA synthesis errors could also be correctly identified. However the approach is less amenable to large scale sequencing projects of high gene diversity and is more suitable for targeted gene variant pools. Although these studies share a similar philosophy to overcome the NGS error-correction issue for the detection of rare variants, our study includes a further restraint in precisely limiting the input tagged template copy number and PCR efficiency during the PCR of step two to accurately control the distribution of cluster count in the sequencing output to a median cluster size of 10 amplicons. Limiting redundancy input in order to minimize unnecessary loss of sequencing capacity is also mentioned in a recent NGS error-correction study by Schmitt et al. where the approach was to independently affix a 12-mer unique sequence tag to both strands of a sheared size-selected targeted sequence DNA . After NGS sequencing and error correction, the approximated error frequency was reported at 3.8 × 10−10, representing a great sensitivity improvement in rare mutation identification. In this approach the target sequence DNA was sheared and size-selected, an approach more suitable for cellular DNA versus short viral genome DNA fragments, as we observe DNA shearing to over-represent DNA termini. As many NGS error-correction methods are currently being reported in the literature, the goals of the experiment must be evaluated and a suitable error-correction approach selected as each has their applications, limitations, and advantages.
Sequencing data analysis
Sequencing reads were mapped by Burrows-Wheeler Alignment tool (BWA) . Custom Python scripts were used to match nucleotide tags, conflate error-corrected amplicon sequences, and other downstream analyses. The mutation frequency after selection was determined by dividing the mutation occurrence by the total population count (WT plus variant), whereas the change in frequency was determined by calculating: [R2 frequency/input frequency] of each mutation.
HIV-1 individual mutant construction
All site directed mutagenesis was conducted with a two-step PCR approach specific to the HIV-1 genomic fragment that contained the targeted substitution. Each substitution and corresponding HIV-1 fragment are as follows: CA A194T:Frag2, PR D25G:Frag3, PR D29G:Frag3, RT E6K:Frag3, RT F61S:Frag3, RT Y501C:Frag4, IN N155Y:Frag4, vif D101N:Frag4, rev E10G:Frag5, gp120 C119G:Frag5, gp120 K205M:Frag5, gp120 D476V:Frag6, gp41 Y136H:Frag6, and 3’LTR C9547T:Frag7. Using 5 ng of pNL4-3 as template, each forward and reverse mutagenic primer was combined with the reverse and forward fragment primers (initially used for error-prone PCR) to generate partial, yet overlapping (at mutagenized codon) PCR fragments of the full sized fragment using high-fidelity KOD DNA polymerase (EMD Millipore) with the cycle parameters 95°C 2 min, 95°C 20 sec, 56°C 20 sec, 68°C 1 min, 30 cycles, 68°C for 10 min, and a final hold at 4°C. Afterwards 5 μL of each purified mutagenic product was combined in a second PCR using the same conditions and cycle parameters with only the forward and reverse fragment primers to generate the full length fragment containing the mutagenized codon. The products were digested with restriction enzymes specific to the fragment: Frag2: BssHII and ApaI, Frag3: ApaI and AgeI, Frag4: AgeI and EcoRI, Frag5: EcoRI and NheI, Frag6: NheI and XhoI, and Frag7: XhoI and NcoI (New England BioLabs), and ligated in correspondingly digested cloning vectors using T4 DNA ligase (Invitrogen) according to manufacturer’s instructions. Mutations were confirmed by sequencing and plasmids were midi-prepped (Invitrogen).
The authors would like to thank Dr. Sam Chow for the CEM T-lymphocyte cell line, and Drs. Matthew Marsden, Jerry Zack, Helen Brown, Martha Lewis, and Otto Yang for helpful discussions concerning HIV-1 biology. This work was supported in part with funds from the UCLA Center for AIDS Research (CFAR) NIH/NIAID AI028697, NIH R21 AI110261, UCLA Jonsson Comprehensive Cancer Center (JCCC) NIH/NCA P30 CA016042, and the California HIV/AIDS Research Program (CHRP) Innovative, Development, Exploratory Award (IDEA).
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