The flow of genetic material between bacteria is central to the adaptation and evolution of bacterial genomes. However, our knowledge about DNA transfer within complex microbiomes is lacking, with most studies of horizontal gene transfer (HGT) relying on bioinformatic analyses of genetic elements maintained on evolutionary timescales or experimental measurements of phenotypically trackable markers. Here, we utilize the CRISPR-Cas spacer acquisition process to detect DNA acquisition events from complex microbiota in real-time and at nucleotide resolution. In this system, an E. coli recording strain is exposed to a microbial sample and spacers are acquired from transferred plasmids and permanently stored in genomic CRISPR arrays. Sequencing and analysis of acquired spacers enables identification of the transferred plasmids. This approach allowed us to identify individual mobile elements without relying on phenotypic markers or post-transfer replication. We found that HGT into the recording strain in human clinical fecal samples can be extensive and is driven by different plasmid types, with the IncX type being the most actively transferred.
Densely populated polymicrobial communities exist ubiquitously in natural environments such as soil and the mammalian gastrointestinal tract. Bacteria in these microbiomes are thought to engage in extensive horizontal gene transfer (HGT) based on metagenomic sequencing studies and comparative genomics analyses1,2,3,4. HGT is a natural phenomenon where DNA is exchanged between organisms through distinct mechanisms including cell-to-cell conjugation of mobile plasmids or genetic elements, transduction by phages and viruses, or transformation by uptake of extracellular nucleic acids5. Upon horizontal transfer, the foreign DNA can be either retained in the recipient or lost over time. HGT processes play a driving role in the evolution of bacterial genomes, leading to the dissemination of important functions such as complex carbohydrate metabolism6, pathogenicity7, and resistance to antibiotics8 or toxic compounds9.
Despite the prevalence of HGT, the evolutionary selection that drives fixation of foreign DNA is generally not well understood; for example, roughly 30% of genes predicted to be acquired by HGT have no known function3, and pan-genome analysis of sequenced genomes predict that many species have open-ended pan-genomes with enormous potential for gene turnover10,11,12. For fixation of transferred DNA to occur in recipient cells many barriers must be overcome, such as specific selection pressures, fitness burden of the acquired element, genetic compatibility with host machinery (e.g., replication, transcription, translation) and presence of anti-HGT systems such as restriction modification systems or CRISPR-Cas systems5,13,14. In addition, the presence of addiction elements on the transferred DNA (e.g., toxin–antitoxin and partitioning systems) also influence the fate of the transferred element. Even when the transferred genetic element provides a fitness benefit they may require many generations to be fixed in a population15. The architecture and dynamics of these gene-flow networks are often not known, especially since most HGT genes are identified from endpoint analyses.
Contemporary computational methods for inferring HGT events rely on different approaches including identification of shared mobile elements such as plasmids or phages, analysis of genomic abnormalities (e.g., shifts in GC% or codon usage) or phylogenetic comparisons between a candidate gene and a conserved gene (e.g., 16 S rRNA)16. On the other hand, experimental approaches to study HGT require the transferred DNA to confer a detectable phenotype that can be enriched in the population. However, not all mobile elements confer a readily selectable phenotype. New selection-independent methods that can capture real-time transfer dynamics across a population will provide a deeper and richer understanding of the overall HGT process.
As a consequence of the pervasive gene flow in microbial genomes, bacteria have evolved various defense systems to manage horizontally acquired genetic material5,17. CRISPR-Cas systems can provide specific and adaptive immunity to invading DNA13,14. During the conserved CRISPR adaptation process, Cas1 and Cas2 proteins capture short fragments of invading DNA and integrate them as spacers into CRISPR arrays13,18, a process that requires active cell division19. In E. coli, immunity is conferred by transcribed spacers guiding the CRISPR-associated complex for antiviral defense (Cascade) to the invading DNA20. Importantly, the CRISPR arrays provide a useful long-term record of horizontally invading DNA.
Different CRISPR-Cas types have been identified across bacterial and archaeal phyla and have been engineered to study spacer adaptation21. Adaptation of new spacers into CRISPR arrays is a rare event under simulated natural conditions13,22, and in contrast to acquired immunity in Streptococcus thermophilus13, most natural E. coli strains do not actively acquire new spacers and their arrays therefore reflect ancient HGT events23. However, spacer acquisition can be stimulated if the CRISPR array is ‘primed’ with a spacer matching the foreign DNA24. Furthermore, heterologous expression of cas1 and cas2 can lead to high levels of spacer adaptation24,25, a process that can be leveraged for engineered signal recording and storage applications26,27,28.
Here, we leverage the CRISPR spacer acquisition process as a mechanism for real-time recording of HGT events at nucleotide-resolution. Using an optimized acquisition system, we can capture transient HGT events and identify DNA transfers that cannot be easily detected with traditional methods. The performance and technical accuracy of this system was rigorously characterized using defined donor strains and communities. Application of the system to clinical human fecal samples revealed prevalent and diverse DNA transfer events, shedding light on the dynamics of HGT in the mammalian gut microbiome into an E. coli recipient.
Identifying exogenous HGT using CRISPR spacer acquisition
We previously engineered a CRISPR-based temporal recording system that acquired new spacers from either endogenous genomic DNA or a copy-number inducible plasmid28. In this system, we utilized a recording strain (hereafter referred to as EcRec) consisting of E. coli BL21 with the pRec-ΔlacI plasmid containing an anhydrotetracycline (ATc) inducible operon of the E. coli Type I-E cas1 and cas2 genes. Upon induction of the recording strain, over-expressed Cas1 and Cas2 proteins incorporate DNA protospacer sequences into CRISPR array I on the genome at high frequencies28. Since E. coli BL21 lacks the Cascade interference machinery, acquired spacers do not lead to CRISPR-mediated adaptive immunity20. The system can thus serve as a recorder of intracellular DNA. CRISPR expansions can be easily analyzed by PCR amplification of the CRISPR array from a population of recording cells, and, if needed, enrichment for arrays with new spacers can be achieved by a simple gel extraction of expanded array products. Subsequent deep amplicon sequencing can be used to assess the spacer repertoire28. While spacers can be acquired from both endogenous and exogenous DNA sources, including the genome, there is a strong preference to acquire spacers from high copy replicative plasmids19,22. Given the capacity of the cas1/cas2 overexpression system to record intracellular DNA at much higher efficiency than the wild-type system, we hypothesized that the system could be used as a sensitive method to reveal HGT events (Fig. 1a) that may only occur transiently or at a low-frequency across a cell population.
To explore whether CRISPR recording can allow direct measurement of HGT events, we exposed the recording strain (EcRec) to the E. coli strain FS1290 that harbors the well-characterized broad host range conjugative plasmid RP4 ref. 29. Before mixing the two strains, expression of cas1 and cas2 was induced to ensure maximum acquisition capacity (see Methods). In addition, non-induced EcRec served as a control. Conjugation was carried out by mixing the strains in a 1:1 ratio and spotting them on agar plates with and without ATc. Reactions without the donor E. coli FS1290 strain served as an additional control. After 6 h, the cells were collected and CRISPR arrays were amplified and sequenced (without gel extraction) to evaluate the spacer repertoire, yielding 104–105 sequenced arrays per biological replicate (Supplementary Data 1). In the cas1/cas2 induced cells with donor, 1.0% (sd = 0.1%, n = 5 recordings) of the arrays were expanded in contrast to only 0.0010% (sd = 0.0006%, n = 5 recordings) in the non-induced cells (Fig. 1b). Further probing of the dynamics of the HGT recording process showed that overall spacer expansion could be identified as early as 1 h after mixing the donor and recording cells, with the rate of array expansion leveling off after 4 to 6 h of conjugation (Fig. 1c). By 24 h, 1.9% of all arrays (sd = 0.5%, n = 5 recordings) were expanded (Supplementary Data 1).
As expected, most spacers were derived from the EcRec genome and pRec plasmid. We therefore applied a stringent two-step filter against a de novo sequenced EcRec/pRec reference to isolate putative exogenous spacer sequences. First, only spacers flanked by the canonical direct repeat sequences were kept. Second, spacers with even moderate sequence homology (≥80% identity and coverage) to the EcRec genome or the pRec plasmid were removed (and Methods and Supplementary Methods). Using these filtering criteria, we found that among the expanded arrays, exogenous spacers constituted up to 30–40% of all new spacers and could be detected within 1 h of conjugation (Fig. 1d). After 24 h, 21% (sd = 5%, n = 5 recordings) of the sequenced spacers were identified as exogenous. The number of exogenous spacers was influenced by the ratio of donor to recording cells, and we could detect new exogenous spacers in as few as 1 donor per 106 recording cells (Supplementary Fig. 1). In comparison, only 0.5% (sd = 0.2%, n = 5 recordings) of the spacers in the induced no-donor experiment were identified as exogenous, likely representing spacer sequences containing technical sequencing errors (Supplementary Data 1).
In complex microbiomes, the identity of potential transferred elements is unknown. However, acquired exogenous spacers can be matched against large sequence databases (e.g., GenBank refseq) to identify specific mobile elements. To define the criteria for a match between a spacer and a reference database, we first gel extracted and sequenced spacers from the 24-h E. coli FS1290 recording samples (Supplementary Data 2). Then, a set of scrambled spacers was generated by randomly reordering the sequence of the exogenous spacers. Using BLAST, both original and scrambled spacers were searched against the Genbank RefSeq bacterial genomes database. We identified a conservative hit-threshold of ≥95% identity and coverage that prevented spurious matches of scrambled spacers to the database (Supplementary Fig. 2). Using this threshold, we found that 98.6% (sd = 0.2%, n = 5) of the unique exogenous spacers could be mapped back to the RP4 plasmid sequence (Fig. 1e) and that spacers were acquired across the plasmid, preferably from sites corresponding to the known PAM recognition sequence of E. coli Cas1/Cas2 (AAG, 50% of all spacers, Supplementary Fig. 3). In addition, we observed increased spacer density between the origin of replication (oriV) and the origin of transfer (oriT) (Fig. 1e). Early work on spacer adaptation has shown that acquisition hotspots exist30 and it has been shown that spacer adaptation is a replication dependent process with increased spacer acquisition at stalling replication forks19. We speculate that single stranded nicks at the oriT site stall the unidirectional replication fork of RP4 ref. 31 causing increased spacer adaption. Together, these results show that the EcRec is capable of recording DNA transfer events robustly with high sensitivity and that exogenous spacers can be confidently mapped to the mobile DNA of origin.
Detection of non-replicative and complex HGT events
Many HGT events may be transient or may occur at low frequencies. We hypothesized that our recording system could capture spacers from HGT events in which the transferred element is not stably maintained in a recipient. To investigate transfer of both genomic DNA and a non-replicative plasmid we used an E. coli S17 strain carrying the R6K-derived plasmid pUT, as the donor32. E. coli S17 contains a genomically integrated copy of the RP4-Tet::Mu conjugation system and also expresses the R6K replication initiation protein Pir. The integrated RP4 can mobilize the S17 genome and the pUT plasmid into recipient cells33. However, pUT requires the Pir protein in trans in order to replicate and therefore cannot be maintained in the EcRec recipient, which lacks the pir gene32,34. In addition, phage Mu, which is also present in S17, can be acquired by recipients either via conjugation of the S17 genome or via phage particles34. We mixed EcRec with the E. coli S17/pUT donor strain and recorded spacers for 6 h. Analysis of new exogenous spacers from the S17/pUT donor showed acquisition from both the integrated RP4-Tet::Mu and the pUT plasmid, highlighting that active replication of the transferred element is not required for spacer acquisition (Fig. 2a). We further investigated whether EcRec could record DNA from infecting M13 phage. As M13 infects cells via the F-pili we first generated a phage susceptible EcRec by conjugating F′ from E. coli K603 into EcRec. Induced EcRec/F′ was exposed to M13 and after 24 h incubation with ATc, and the arrays were amplified and sequenced. We found six spacers acquired from M13 (Supplementary Fig. 4), showing that recording of this phage was possible although with a low efficiency. Previous work studying spacer acquisition from infecting M13 in Cascade proficient E. coli found a 3% acquisition rate amongst isolates selected for their resistance to phages using a multiplicity of infection (MOI) of 10 ref. 24. The low adaptation rate in our study, even in the background of cas over expression, may be caused by the reduced growth rate the infected cells35. We also attempted to detect transfer of the Gram-positive mobile plasmids pGO400 and pSL20 from S. aureus and B. subtilis, respectively, but we could not detect any spacers. We speculated that this might be due to the plasmids not entering the recording cells. To test this, we electroporated the plasmid DNA into the recording cells, in these cases we were able to detect spacers at low frequencies from electroporated plasmid as well as S. aureus and B. subtilis chromosome (Supplementary Fig. 5).
Since natural bacterial isolates often carry multiple plasmids capable of transfer, we tested if our recording system could resolve transfer of different mobile elements from the same donor. A clinical E. coli isolate (Ec70) that carried 6 different plasmids (p1–p6), as resolved by hybrid assembly (Oxford Nanopore and Illumina sequencing, Methods), was used as the donor strain (Supplementary Data 3). Sequencing and analysis of new spacers from a recording experiment with Ec70 revealed that 97% of exogenous spacers were acquired from only two plasmids, the 55 kb plasmid p4 and the 4 kb plasmid p6. We quantified the spacer mapping to the reference sequence as the average number of spacers per kb per 1000 exogenous spacers, hereafter referred to as normalized spacer mapping (Fig. 2b). The normalized spacer mapping of each plasmid provides a semi-quantitative estimate of its relative transfer frequency, however, variations in PAM-site frequency and plasmid copy number will affect the estimates.
For p4 and p6 the normalized spacer mapping was 13.5 (sd = 0.4), and 6.0 (sd = 0.8), respectively (n = 5). While plasmid p4 is self-transmissible, the much smaller plasmid p6 only carries the mobilization protein MobA, hence requiring the conjugation apparatus in trans. Neither of the two plasmids carry any antibiotic resistance genes highlighting that our recording system can readily detect elements that would not be easily detectable by standard selection-based methodologies. Plasmids p3 and p5 (80 kb and 33 kb, respectively) appeared to transfer, although at very low frequencies with a normalized spacer mapping of 0.060 and 0.48, respectively (sd = 0.03 and 0.15, n = 5 recordings). No spacers were observed from the 106 kb large plasmid p1 and only eight spacers were observed from the 102 kb plasmid p2 (Fig. 2b) from a total of ~1 million expanded spacers. As expected, spacers were acquired from across the plasmid backbones (Fig. 2c). These results demonstrate that CRISPR-based recording of HGT can reveal and resolve the transfer dynamics of different mobile elements from a donor carrying 6 plasmids.
Capturing HGT events from a defined microbial community
Having characterized the recording system using a single donor, we explored whether HGT events could be recorded in a complex, multi-donor community. A defined bacterial community comprised of 6 clinical E. coli isolates (Ec77, Ec70, Ec35, Ec14, Ec75, Ec21) as well as a positive control strain (FS1290) that carries the RP4 plasmid, and a negative control strain (REL606) that contains no plasmids was assembled. We generated draft genome assemblies and predicted that the clinical E. coli strains carried at least two plasmids each, including Ec70 already established to carry six plasmids36 (Fig. 3, Supplementary Data 3).
Donor strains were pooled in equal ratios and then mixed with EcRec. The recording was carried out for 6 h on LB agar + ATc and new exogenous spacers were identified and mapped back to the contigs from the draft genome assemblies for each of the 7 donor strains while the hybrid assembly was used for Ec70 strain. Spacers mapping to more than one contig were filtered out to ensure an unambiguous interpretation of HGT events (26.0%, n = 3205). We detected new spacers from all donor strains except from the negative control REL606 (Fig. 3). However, spacers were not acquired equally from the donors, with 72% (sd = 9%, n = 5 recordings) of all spacers deriving from the FS1290 positive control strain, confirming that RP4 transfers at high frequency37. Clinical strains Ec77 and Ec70 were particularly efficient donors, representing 19% and 7.3% of total spacers, respectively (sd = 9% and 2.4%, n = 5 recordings). Based on this mapping, we could also identify which predicted plasmids were being transferred. For instance, IncFII-type plasmids in Ec35, Ec75, Ec77 appear to transfer readily to EcRec, while col-type plasmids in Ec21, Ec75, and Ec77 do not appear to mobilize. Importantly, we qualitatively detect the same transfer profile for Ec70 in this community recording as in the single donor recording. However, all spacers mapping to the IncX3 plasmid in Ec70 were removed due to redundant mapping to other plasmids in the community.
Capturing HGT events from natural microbial communities
Extensive HGT has been reported in the human microbiome and has been shown to facilitate the spread of clinically important genes such as antibiotic resistance genes3,4,38,39,40. Therefore, we sought to identify mobile DNA accessible to E. coli in clinically relevant human fecal microbiomes. Fecal samples were from hospitalized adults with diarrhea whose stools were tested for Clostridium difficile infection (CDI). Of 27 patient-samples, 24 had received broad-spectrum antibiotic treatment in the month prior to sampling while the remaining (FS05, FS06, and FS07) did not receive antibiotics. For each sample, ~0.5 g of fecal matter was washed in PBS three times to remove potential inhibiting compounds, such as antibiotics. The washed samples were each mixed with pre-induced EcRec, spotted on LB agar + ATc, and incubated for 24 h. In order to confidently identify samples with HGT events we established strict criteria requiring that at least 10 exogenous spacers were identified and that the percentage of exogenous spacers was at least 3 times higher than in the no-donor control samples (0.03%). From the 27 recordings, we sequenced >10 million CRISPR arrays (Fig. 4a). Six recordings passed our criterion representing a total of 20,991 exogenous spacers yielding 5686 unique spacers (Supplementary Data 2). To investigate the reproducibility of the fecal recordings, we repeated the recording for three samples that had a high number of exogenous spacers (FS01-03) and three samples with a low number of exogenous spacers (FS10-12). We found that the overall within-sample reproducibility was high and that the samples were clearly delineated into the initial groups of high and low numbers of exogenous spacers (Supplementary Fig. 6). Furthermore, we investigated how sequencing depth affected the number of exogenous spacers and we saw no correlation between sequencing depth and the number of exogenous spacers within the six samples with HGT events (Supplementary Fig. 7).
We hypothesized that the presence of closely related donor species would be important to observing HGT. We thus profiled the composition of all 27 fecal samples using 16 S rRNA amplicon sequencing (Fig. 4b). Overall, the α-diversity (number of species) was similar regardless of whether or not high numbers of exogenous spacers were observed (Fig. 4b, c). However, as predicted, we found that the relative abundance of the Escherichia/Shigella taxa (Otu1) was significantly elevated in the 6 samples passing the recording criteria (Fig. 4d, p = 0.0070, two sided Mann–Whitney U test). Still, some samples with high abundance of Escherichia/Shigella had few exogenous spacers (e.g., FS09 and FS14), suggesting that presence of Escherichia/Shigella at high abundance is correlated with but not sufficient for detectable transfer (e.g., presence and mobilization of plasmids may be variable or bacteriocins production might inhibit EcRec).
To identify the source of exogenous spacers, we used BLAST to search the NCBI RefSeq bacterial genome database, NCBI RefSeq viral genome database and a custom plasmid database applying the previously established thresholds (Methods). Overall, the majority of the 5686 unique exogenous spacers could be matched to at least one of the databases (Supplementary Data 2). All spacers with hits to the viral database also matched to the genome database. Furthermore, > 95% of spacers with hits to the genome database also matched to the plasmid database, highlighting that the identifiable spacers were most likely of plasmid origin. For each sample, we identified the minimal set of reference plasmids that encompass all spacers. Clustered heatmaps from these plasmid hits were used to identify the likely source plasmid of the exogenous spacers and predict the number of discrete mobile genetic elements recorded from the sample. For each sample, we infer that 1–2 different plasmids were transferred (Fig. 5a).
For instance, BLAST hits of spacers to the plasmid database in sample FS02 indicate that two plasmids were transferred, a large IncX-type plasmid and a small colE-type plasmid (Fig. 5a). The putative IncX hits match to a 35 kb plasmid (Genbank accession CP004088) carrying no resistance markers. The acquired spacers map across the entire plasmid back-bone, suggesting that the reference is a good representation of the transferred plasmid. The small colE-like plasmid (Genbank accession CP003036) has three predicted open reading frames (ORFs): a replication protein, a mobilization protein and an unknown ORF. While spacer coverage of the colE plasmid is sparser than the IncX plasmid, spacers matched across the back-bone suggesting that all regions of the pCE10B plasmid were present in the mobilized plasmid captured from FS02. Interestingly, the smaller plasmid does not encode a conjugation apparatus and therefore requires conjugation genes in trans for mobilization. Mapping all acquired spacers to the Plasmid Finder database36 revealed matches to IncX, IncI, IncF, IncH, pO157_Sal, and colE plasmid types, which are all common replicons in Enterobacteriaceae (Fig. 5a).
To better delineate the functions of the ORFs that yielded spacers, we used the RefSeq database to extract the functional annotations of genes with spacer hits (Fig. 5b and Supplementary Data 4). For each sample, 80–85% of spacers had functional annotations. The most common gene annotations were associated with canonical plasmid functions including conjugation, replication and plasmid addiction genes. As expected, a large portion of the ORFs had no known function (Fig. 5b). Given that the majority of patients received antibiotics recently (4/6 with detectable transfer), one might expect that the transferrable plasmids would harbor antibiotic resistance genes. However, mapping of spacers to the ResFinder database41 yielded only two spacer hits to antibiotic resistance genes, a blaTEM beta-lactamase and a chloramphenicol acetyltransferase gene (both from FS04), suggesting that, although present, resistance genes are not particularly abundant in the pool of mobile plasmid that can move into EcRec, even after extensive antibiotic treatment.
Identification of transferred plasmids from metagenomes
We further performed shotgun metagenomic sequencing on the original fecal samples to assess the recovery of spacers against assembled contigs and to confirm the presence of putative plasmids in the samples. Metagenomic reads were assembled yielding ~371 Mbps of contigs across the six samples with observed plasmid transfer events (FS01-FS06) (Supplementary Data 5). Most acquired spacers could be matched to metagenomic contigs by BLAST (Fig. 6a). However, in two samples, FS05 and FS06, the metagenomic recovery rate was very low (3% and 8%, respectively). Correspondingly, these samples also had few acquired unique exogenous spacers (112 and 36, respectively), suggesting low frequency of HGT. Mapping of all exogenous spacers to the plasmid database revealed that the majority of spacers matched to both metagenomic contigs and published plasmids, confirming that most transfer was via plasmids (Fig. 6a).
Using the Plasmid Finder database36, we identified putative plasmid contigs across the metagenomes. We observed transfer of a variety of Enterobacteriaceae plasmids including IncF, IncX, IncI, and col types, corroborating the results generated with our plasmid database (Fig. 6b). In addition, we also detected a number of non-transferred plasmids (e.g., repUS2) from Gram-positive species including S. aureus. Interestingly, certain plasmid types appeared to transfer more readily than others based on comparing their spacer mapping density and metagenomic coverage. In particular, IncX-type plasmids transferred efficiently since we observed similar spacer mapping densities across three orders of magnitude in metagenomic coverage (Fig. 6b, FS01, FS02, and FS04). In contrast, IncI-type plasmids transferred at very low levels despite the metagenomic coverage varying two orders of magnitude between FS01 and FS02 (Fig. 6b).
In some cases, spacers mapped only to the metagenomic contigs (and not to the plasmid database; Fig. 6a and Supplementary Fig. 8). Among those contigs, contig 137 (21 kbp) from FS01 had a majority of metagenome-only spacers (202/276) indicating that the contig was not normally found on plasmids (Fig. 6c). This contig consisted of a region encoding a P-type fimbria along with a transposase as well as a region containing hypothetical proteins. The former region has been found in other plasmids, as indicated by spacer mapping to the plasmid database, while the latter region appears to be specific to the FS01 sample (Fig. 6c). The contig is not classified as plasmid, however, it is likely an incomplete assembly of a larger plasmid. Online BLAST of the contig against the nt database confirmed that there were no hits with broad coverage, and the best hit was an unnamed E. coli plasmid with 27% coverage at 92% identity to contig 137. This highlights the utility of our approach to identify novel transferred elements that may not be predicted by traditional reference-based methodologies.
Comparative analyses of sequenced genomes have provided important insight into the HGT processes3,4 occurring in different complex environments3,4. Our CRISPR-based recording system adds more detailed insights into the dynamics of HGT in complex environments by detecting DNA transfer events as they occur, enabling detection of transient transfer events.
The recording system captures spacers from HGT events stably into genomic arrays that can be used to identify mobile elements beyond current methodologies. The ability to detect, in real-time, transient transfer events and those occurring at low frequencies enables an in-depth characterization of mobile DNA in complex microbiomes.
As DNA transfer is confined by recipient range we are only capable of recording DNA that can enter the E. coli BL21 recording strain. When using other E. coli strains as donor we showed that transfers can be resolved down to the individual plasmids from donors that can carry up to 6 putatively mobile plasmids. We find that the different plasmids varied in transfer efficiencies likely reflecting differences in intrinsic plasmid transfer efficiency, donor transfer efficiency, recipient receiving efficiency, or a combination of these factors. Even though the observed mobile elements were all classified as plasmids, we still expect that phages are an important contributor to HGT. However, as illustrated by the recording of phage M13, our system is not optimal for detecting invading phages as CRISPR spacer adaptation requires active growth of the recording cell19, which is often impaired upon phage infection. In addition, infection with phages can lead to cell lysis and subsequent loss of recording cells from the population. Furthermore, it is not clear what the expected concentration of E. coli targeting phages is in human fecal samples. Previous studies indicate that plaque forming units (pfu) from human feces on E. coli is in the range of 101–107 per gram, with a median concentration of ~103 per gram42,43. Considering that the concentration of E. coli in human feces is in the range of 107–109 per gram44, interactions between phages and the recording strain might be substantially less common than interactions between commensal E. coli and the recording strain. Washing of the fecal sample (i.e., to remove antibiotics and other factors that can inhibit the recording strain) likely also contributed to the loss of phage particles. Lastly, as E. coli is not naturally competent, we are not able to detect ‘naked’ environmental DNA. Consequently, our recording strain is best suited for detecting plasmid transfers.
When our approach is applied to clinical fecal specimens, we were able to identify active DNA transfer in 22% of the samples (6 out of 27). It is difficult to evaluate whether the frequency of observed HGT in the fecal samples (22%) is limited by the methodology or whether it reflects the enterobacterial transfer capacity of these samples. As the fecal recordings were performed aerobically, our approach was only able to capture transfers from aerobically active donors, potentially limiting some transfers. Additionally, the potential presence of bacteriocin producing strains could limit the growth of EcRec and hence lead to fewer acquired spacers. Yet, across the six metagenomes, the number of different plasmid replicons present varied greatly (Fig. 6b), suggesting that some samples contained fewer plasmids. In many instances, we observed multiple discrete plasmids being transferred, most of which did not carry selectable markers such as antibiotic resistance genes indicating that a substantially larger pool of active and mobile plasmids exists in the gut microbiome beyond just the antibiotic resistance plasmids that are typically identified by phenotypic assays.
By analyzing the captured spacers, we also found that many horizontally acquired genes have no known function, in agreement with previous bioinformatic analyses3. Using metagenomic sequencing, we definitively matched acquired spacer sequences to assembled plasmid contigs and plasmid types involved in these HGT events. While many different plasmids were identified in the metagenome, only subsets were shown to mobilize into EcRec, with the IncX type transferring most efficiently.
In the current system, spacer acquisition is driven by overexpression of cas1 and cas2, yet after 24 h induction only about 2% of arrays are expanded, limiting the recording capacity and sensitivity of the system. Increasing the array expansion rate would improve the spacer output relative to sequencing depth and help improve sensitivity. However, the vast majority of spacers are acquired from endogenous sources, and it would therefore be desirable to increase the ratio of exogenous spacers to total spacers. Including an active Cascade complex could help counter select endogenous spacers, although, as many arrays adapt multiple spacers, it could potentially affect recording sensitivity.
Endogenous or engineered Cas1/Cas2 recording systems could be implemented in the context of different hosts to understand the host specificity of transfer for diverse bacterial species. These various systems and hosts could be multiplexed for high-resolution recording of HGT in various environments, from the human gut to various environmental microbiota. This would enable real-time recording of previously difficult-to-record transient HGT events, and offers a powerful new approach to studying flow and transfer of mobile DNA at an unprecedented resolution.
The recording strain (EcRec) was BL21 (NEB C2530H) with the pRec ΔlacI plasmid (Addgene #104575)28. Clinical E. coli isolates were a kind gift from Dr. Kristian Schønning, Hvidovre Hospital, Denmark. See Supplementary Data 6 for full overview of donor strains.
All strains were grown in LB medium with appropriate antibiotics and washed in PBS prior to recording. In all recordings an overnight culture of the recording strain was diluted 1:50 and grown for one hour, then anhydrotetracycline (ATc) was added to a final concentration of 100 ng/mL and the strain was incubated for another hour. Next, the recording strain and the donor strain were washed to remove antibiotics and resuspended in LB + aTc 100 ng/ml. The recording strain and donor strain were mixed 1:1 at OD600 = 0.5, except in the ratio experiment (Supplementary Methods) where strains were mixed in the ratios described in the figure. After mixing, the mixture was spotted on LB agar + 100 ng/mL aTc. Plates were incubated for 6 h at 37 °C. At the end of a recording, the cells were scraped off the plate and resuspended in 100 µl PBS and heat inactivated at 95 °C. for 3 min, subsequently they were stored at −20 °C until sequencing analysis.
Recording of phage M13
Phage particles were generated by electroporating phage M13 DNA (NEB M13KE) into E. coli K603 and growing the strain to saturation in 10 ml LB followed by sterile filtration of the supernatant. The number of plaque forming units (pfu) was determined using the NEB protocol ‘M13 Titer Protocol’ (https://www.neb.com/protocols/2014/05/08/m13-titer-protocol) using EcRec/F’ as the indicator strain. Recording of M13 was done in LB with pre-induced EcRec/F’ at a concentration of 106/ml and adding M13 at a multiplicity of infection (MOI) of 100. Recording was carried out for 24 h.
The donor strain was prepared as described above. All fecal recordings were performed on fresh fecal samples (collected within 24 h of the recording). For each sample ~0.5 g were washed 2 times in 1 ml PBS and finally resuspended in 100 µl LB + 100 ng/ml ATc. The washed fecal sample was mixed with a 100 µl resuspension of 1 ml OD600 = 0.5 of the recording strain. From this mixture 50 µl was plated on LB agar + 100 ng/ml ATc and incubated for 24 h at 37 °C aerobically. Subsequently, the samples were processed as described above.
The protocol for the collection of human samples and data was approved by the Columbia University Medical Center Institutional Review Board with a waiver of informed consent (IRB AAAR9489). Residual (waste) fecal specimens were used following standard clinical testing, and anonymized data was retrieved retrospectively.
CRISPR arrays were sequenced utilizing our established sequencing pipeline28 with minor modification. Briefly, DNA from cells was obtained by enzymatic and heat lysis, barcoded PCR amplification of CRISPR arrays was performed samples were pooled and sequencing was performed on the Illumina MiSeq platform (MiSeq v2 50 cycle, MiSeq v2 300 cycle or MiSeq v3 150 cycle kits) with additional spike-in of custom sequencing primers (for primer list see ref. 28). In addition, to enrich for expanded spacers, double gel extraction of expanded spacer bands on an E-gel EX Agarose Gel 2% was performed on pooled libraries. An overview of sequencing runs and sample statistics can be found in Supplementary Data 1, 2, 5
Spacers were extracted utilizing our established spacer extraction pipeline; code can be accessed at https://github.com/ravisheth/trace. Extracted spacers were filtered against the genome of the recording strain (quality filtered reads from sequencing of the same EcRec BL21/pRecΔlacI) using a two-step process using USEARCH v10.0.240 ref. 45. First spacers were filtered using a database of word size 8, then all non-hit spacers were collected and filtered against the same database using word size 5 (e.g., ‘usearch -usearch_global -id 0.8 -query_cov 0.8 -top_hit_only -maxrejects 0 -strand both -uc out.uc’). Subsequently the identified exogenous spacers were uniqued e.g.,(‘usearch -fastx_uniques -fastaout centroids.fa -sizeout’). The unique exogenous spacers was utilized in all subsequent spacer mapping performed with BLAST 2.7.1 + (‘blastn -db -query -perc_identity 90 -max_target_seqs 500000000 -task blastn -word_size 10 -outfmt “6 std sstrand qlen slen”). The output of BLAST was filtered to ensure 95% identity and 95% coverage of the query spacer. An example of the processing workflow can be seen in Supplementary Methods. Data analysis was performed in R46 using ggplot2 ref. 47 and CLC main workbench (www.qiagenbioinformatics.com).
The following reference databases were used to identify the source of the acquired spacers: Prokaryotic RefSeq Genomes from January 2018; ftp://ftp.ncbi.nlm.nih.gov/genomes/refseq/bacteria/. Viral RefSeq Genomes from January 2018; ftp://ftp.ncbi.nlm.nih.gov/genomes/refseq/viral/. A custom plasmid database was created using the following search criteria in NCBI GenBank nucleotide database from January 2018; ‘plasmid[TI]’, then summary file was downloaded and parsed to get accession numbers of all circular elements:
‘grep -A1 ‘bp circular DNA’ summary.txt | grep -v ‘bp circular DNA’ | grep -v ‘\-\-‘ | cut -d’ ‘ -f1 > output.txt’ which were subsequently retrieved with NCBI batch (https://www.ncbi.nlm.nih.gov/sites/batchentrez).
16 S rRNA sequencing
16 S rRNA sequencing was performed utilizing our established sequencing pipeline; detailed methods can be found in our previous publication48. Briefly, genomic DNA (gDNA) was extracted with a protocol utilizing the Qiagen MagAttract PowerMicrobiome DNA/RNA kit (Qiagen 27500-4-EP). Samples were bead beat with 0.1 mm Zirconia Silica Beads (Biospec 11079101Z) for a total of ten minutes (Biospec 1001); the Qiagen kit protocol was followed but at reduced volumes on a Biomek 4000 liquid handling robot. The resulting gDNA was subjected to 16 S V4 amplicon sequencing utilizing custom barcoded primers49 and NEBNext Q5 Hot Start HiFi Master Mix (NEB M0543L). Resulting PCR products were quantified and pooled on a Biomek 4000 robot and sequenced utilizing an Illumina MiSeq V2 300 cycle kit. The sequencing data was analyzed using USEARCH 10.0.240 ref. 45; reads were merged (-fastq_mergepairs), filtered (-fastq_filter -fastq_maxee 1.0 -fastq_minlen 240), and 100% ZOTUs were generated (-unoise3) and OTU table created (-otutab). Taxonomy was assigned to ZOTUs using the RDP classifier50. The OTU table was rarefied to 1000 reads per sample before analysis.
Whole genome and shotgun metagenomic sequencing
The recording strain BL21/pRec along with all donor strains were subjected to whole genome sequencing (Supplementary Data 6) and clinical samples were subjected to shotgun metagenomic sequencing (Supplementary Data 5). gDNA was extracted from individual isolates or fecal samples utilizing the gDNA extraction pipeline detailed above. Sequencing preparation followed a published protocol for low-volume Nextera library preparation51. Barcoded samples were pooled and sequencing was performed on the Illumina MiSeq (2 × 150 reads), Illumina NextSeq (2 × 75 reads) or Illumina HiSeq X platform (2 × 150 reads). Adapters were trimmed utilizing Trimmomatic52. Draft assemblies for the donor strains were conducted using SPAdes utilizing the --careful flag53. Metagenomes were assembled with SPAdes utilizing the --meta flag. Raw metagenomic reads were mapped to the refseq viral database as well as the plasmid database using bwa mem54.
The donor strain Ec70 was further sequenced utilizing the Oxford MinION platform; genomic DNA was extracted with a Gentra Puregene kit (Qiagen), prepared for sequencing utilizing the RAD004 kit and sequenced on a single R9.4.1 flow cell. For this strain, hybrid assembly of the genome and individual plasmids was conducted utilizing UniCycler55. See Supplementary Data 6 for genome sequencing information and Supplementary Data 5 for metagenome sequencing information.
Further information on research design is available in the Nature Research Reporting Summary linked to this article.
Assembled genomes, metagenomic reads, and CRISPR array sequencing data is deposited under bioproject number PRJNA594543. All other relevant data are available from the corresponding author upon request.
Shoemaker, N., Vlamakis, H., Hayes, K. & Salyers, A. Evidence for extensive resistance gene transfer among bacteroides spp. and among bacteroides and other genera in the human colon. Appl. Environ. Microbiol. 67, 561–568 (2001).
Coyne, M. J., Zitomersky, N., McGuire, A., Earl, A. M. & Comstock, L. E. Evidence of extensive DNA transfer between bacteroidales species within the human gut. mBio 5, e01305–e01314 (2014).
Brito, I. et al. Mobile genes in the human microbiome are structured from global to individual scales. Nature 535, 435 (2016).
Smillie, C. S. et al. Ecology drives a global network of gene exchange connecting the human microbiome. Nature 480, 241 (2011).
Thomas, C. M. & Nielsen, K. M. Mechanisms of, and barriers to, horizontal gene transfer between bacteria. Nat. Rev. Microbiol. 3, 711–721 (2005).
Hehemann, J.-H. et al. Transfer of carbohydrate-active enzymes from marine bacteria to Japanese gut microbiota. Nature 464, 908 (2010).
Schmidt, H. & Hensel, M. Pathogenicity islands in bacterial pathogenesis. Clin. Microbiol. Rev. 17, 14–56 (2004).
Wellington, E. M. et al. The role of the natural environment in the emergence of antibiotic resistance in Gram-negative bacteria. Lancet Infect. Dis. 13, 155–165 (2013).
Martinez, R. J. et al. Horizontal gene transfer of PIB-Type ATPases among bacteria isolated from radionuclide- and metal-contaminated subsurface soils. Appl. Environ. Microbiol. 72, 3111–3118 (2006).
Tettelin, H. et al. Genome analysis of multiple pathogenic isolates of Streptococcus agalactiae: Implications for the microbial “pan-genome”. Proc. Natl Acad. Sci. USA 102, 13950–13955 (2005).
Rasko, D. A. et al. The pangenome structure of Escherichia coli: comparative genomic analysis of E. coli commensal and pathogenic isolates.J. Bacteriol. 190, 6881–6893 (2008).
Lapierre, P. & Gogarten, P. J. Estimating the size of the bacterial pan-genome. Trends Genet. 25, 107–110 (2009).
Barrangou, R. et al. CRISPR provides acquired resistance against viruses in prokaryotes. Science 315, 1709–1712 (2007).
Marraffini, L. A. & Sontheimer, E. J. CRISPR interference limits horizontal gene transfer in staphylococci by targeting DNA. Science 322, 1843–1845 (2008).
Nielsen, K. M. & Townsend, J. P. Monitoring and modeling horizontal gene transfer. Nat. Biotechnol. 22, 1110–1114 (2004).
Ravenhall, M., Škunca, N., Lassalle, F. & Dessimoz, C. Inferring horizontal gene transfer. PLoS Comput. Biol. 11, e1004095 (2015).
Koonin, E. V., Makarova, K. S. & Wolf, Y. I. Evolutionary genomics of defense systems in archaea and bacteria. Annu. Rev. Microbiol. 71, 1–29 (2016).
Sorek, R., Lawrence, M. C. & Wiedenheft, B. CRISPR-mediated adaptive immune systems in bacteria and archaea. Biochemistry 82, 237–266 (2013).
Levy, A. et al. CRISPR adaptation biases explain preference for acquisition of foreign DNA. Nature 520, 505 (2015).
Brouns, S. J. et al. Small CRISPR RNAs guide antiviral defense in prokaryotes. Science 321, 960–964 (2008).
Sternberg, S. H., Richter, H., Charpentier, E. & Qimron, U. Adaptation in CRISPR-Cas systems. Mol. Cell 61, 797–808 (2016).
Díez-Villaseñor, C., Guzmán, N. M., Almendros, C., García-Martínez, J. & Mojica, F. J. CRISPR-spacer integration reporter plasmids reveal distinct genuine acquisition specificities among CRISPR-Cas I-E variants of Escherichia coli. RNA Biol. 10, 792–802 (2013).
Touchon, M. et al. CRISPR distribution within the Escherichia coli species is not suggestive of immunity-associated diversifying selection. J. Bacteriol. 193, 2460–2467 (2011).
Datsenko, K. A. et al. Molecular memory of prior infections activates the CRISPR/Cas adaptive bacterial immunity system. Nat. Commun. 3, 945 (2012).
Yosef, I., Goren, M. G. & Qimron, U. Proteins and DNA elements essential for the CRISPR adaptation process in Escherichia coli. Nucleic Acids Res. 40, 5569–5576 (2012).
Schmidt, F., Cherepkova, M. Y. & Platt, R. J. Transcriptional recording by CRISPR spacer acquisition from RNA. Nature 562, 380–385 (2018).
Shipman, S. L., Nivala, J., Macklis, J. D. & Church, G. M. Molecular recordings by directed CRISPR spacer acquisition. Science 353, aaf1175 (2016).
Sheth, R. U., Yim, S., Wu, F. L. & Wang, H. H. Multiplex recording of cellular events over time on CRISPR biological tape. Science 358, 1457–1461 (2017).
Datta, N., Hedges, R., Shaw, E., Sykes, R. & Richmond, M. Properties of an R factor from Pseudomonas aeruginosa. J. Bacteriol. 108, 1244–1249 (1971).
Paez-Espino, D. et al. Strong bias in the bacterial CRISPR elements that confer immunity to phage. Nat. Commun. 4, 1430 (2013).
Meyer, R. J. & Helinski, D. R. Unidirectional replication of the P-group plasmid RK2. Biochem. Biophys. Acta 478, 109–113 (1977).
Herrero, M., de Lorenzo, V. & Timmis, K. Transposon vectors containing non-antibiotic resistance selection markers for cloning and stable chromosomal insertion of foreign genes in gram-negative bacteria. J. Bacteriol. 172, 6557–6567 (1990).
Simon, R., Priefer, U. & Pühler, A. A broad host range mobilization system for in vivo genetic engineering: transposon mutagenesis in gram negative bacteria. Nat. Biotechnol. 1, 784 (1983).
Ferrières, L. et al. Silent mischief: bacteriophage Mu insertions contaminate products of Escherichia coli random mutagenesis performed using suicidal transposon delivery plasmids mobilized by broad-host-range RP4 conjugative machinery. J. Bacteriol. 192, 6418–6427 (2010).
Wan, Z. & Goddard, N. L. Competition between conjugation and M13 phage infection in Escherichia coli in the absence of selection pressure: a kinetic study. G3 2, 1137–1144 (2012).
Carattoli, A. et al. In silico detection and typing of plasmids using plasmidfinder and plasmid multilocus sequence typing. Antimicrob. Agents Chemother. 58, 3895–3903 (2014).
Bradley, D., Taylor, D. & Cohen, D. Specification of surface mating systems among conjugative drug resistance plasmids in Escherichia coli K-12. J. Bacteriol. 143, 1466–1470 (1980).
Lester, C. H., Frimodt-Møller, N., Sørensen, T., Monnet, D. L. & Hammerum, A. M. In vivo transfer of the vanA resistance gene from an Enterococcus faecium isolate of animal origin to an E. faecium isolate of human origin in the intestines of human volunteers. Antimicrob. Agents Chemother. 50, 596–599 (2006).
Gumpert, H. et al. Transfer and persistence of a multi-drug resistance plasmid in situ of the infant gut microbiota in the absence of antibiotic treatment. Front. Microbiol. 8, 1852 (2017).
Porse, A. et al. Genome dynamics of Escherichia coli during antibiotic treatment: transfer, loss, and persistence of genetic elements in situ of the infant gut. Front. Cell. Infect. Microbiol. 7, 126 (2017).
Zankari, E. et al. Identification of acquired antimicrobial resistance genes. J. Antimicrob. Chemother. 67, 2640–2644 (2012).
Dhillon, T., Dhillon, E., Chau, H., Li, W. & Tsang, A. Studies on bacteriophage distribution: virulent and temperate bacteriophage content of mammalian feces. Appl. Environ. Microbiol. 32, 68–74 (1976).
Martinez-Castillo, A., Quirós, P., Navarro, F., Miró, E. & Muniesa, M. Shiga Toxin 2-encoding bacteriophages in human fecal samples from healthy individuals. Appl. Environ. Microbiol. 79, 4862–4868 (2013).
Tenaillon, O., Skurnik, D., Picard, B. & Denamur, E. The population genetics of commensal Escherichia coli. Nat. Rev. Microbiol. 8, 207 (2010).
Edgar, R. C. Search and clustering orders of magnitude faster than BLAST. Bioinformatics 26, 2460–2461 (2010).
R Core Team. R: a language and environment for statistical computing.Version 3.6.2 (2019).
Wickham, H. in ggplot2.3–10 (Springer, 2016).
Ji, B. W. et al. Quantifying spatiotemporal variability and noise in absolute microbiota abundances using replicate sampling. Nat. Methods 16, 731–736 (2019).
Kozich, J. J., Westcott, S. L., Baxter, N. T., Highlander, S. K. & Schloss, P. D. Development of a dual-index sequencing strategy and curation pipeline for analyzing amplicon sequence data on the miseq illumina sequencing platform. Appl. Environ. Microbiol. 79, 5112–5120 (2013).
Wang, Q., Garrity, G. M., Tiedje, J. M. & Cole, J. R. Naïve Bayesian classifier for rapid assignment of rRNA sequences into the new bacterial taxonomy. Appl. Environ. Microbiol. 73, 5261–5267 (2007).
Baym, M. et al. Inexpensive multiplexed library preparation for megabase-sized genomes. PLoS ONE 10, e0128036 (2015).
Bolger, A. M., Lohse, M. & Usadel, B. Trimmomatic: a flexible trimmer for Illumina sequence data. Bioinformatics 30, 2114–2120 (2014).
Bankevich, A. et al. SPAdes: a new genome assembly algorithm and its applications to single-cell sequencing. J. Comput Biol. 19, 455–477 (2012).
Li, H. Aligning sequence reads, clone sequences and assembly contigs with BWA-MEM. Preprint at arXiv https://arxiv.org/abs/1303.3997v2 (2013).
Wick, R. R., Judd, L. M., Gorrie, C. L. & Holt, K. E. Unicycler: Resolving bacterial genome assemblies from short and long sequencing reads. PLoS Comput. Biol. 13, e1005595 (2017).
We thank members of the Wang lab for helpful scientific discussions and feedback. H.H.W. acknowledges specific funding from ONR (N00014-17-1-2353), NSF (MCB‐1453219), and NIH (1R01AI132403-01). C.M. acknowledges funding from the Carlsberg Foundation. R.U.S. is supported by a Fannie and John Hertz Foundation Fellowship and a NSF Graduate Research Fellowship (DGE-1644869). C.M. thanks Dr. Kristian Schønning, Hvidovre Hospital, Denmark, for.pngting the clinical E. coli strains.
H.H.W. is a scientific advisor to SNIPR Biome. The remaining authors declare no competing interests.
Peer review information Nature Communications thanks the anonymous reviewers for their contribution to the peer review of this work.
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Munck, C., Sheth, R.U., Freedberg, D.E. et al. Recording mobile DNA in the gut microbiota using an Escherichia coli CRISPR-Cas spacer acquisition platform. Nat Commun 11, 95 (2020). https://doi.org/10.1038/s41467-019-14012-5