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PLoS Genet. Jul 2010; 6(7): e1001017.
Published online Jul 8, 2010. doi:  10.1371/journal.pgen.1001017
PMCID: PMC2900299

A Forward-Genetic Screen and Dynamic Analysis of Lambda Phage Host-Dependencies Reveals an Extensive Interaction Network and a New Anti-Viral Strategy

Ivan Matic, Editor

Abstract

Latently infecting viruses are an important class of virus that plays a key role in viral evolution and human health. Here we report a genome-scale forward-genetics screen for host-dependencies of the latently-infecting bacteriophage lambda. This screen identified 57 Escherichia coli (E. coli) genes—over half of which have not been previously associated with infection—that when knocked out inhibited lambda phage's ability to replicate. Our results demonstrate a highly integrated network between lambda and its host, in striking contrast to the results from a similar screen using the lytic-only infecting T7 virus. We then measured the growth of E. coli under normal and infected conditions, using wild-type and knockout strains deficient in one of the identified host genes, and found that genes from the same pathway often exhibited similar growth dynamics. This observation, combined with further computational and experimental analysis, led us to identify a previously unannotated gene, yneJ, as a novel regulator of lamB gene expression. A surprising result of this work was the identification of two highly conserved pathways involved in tRNA thiolation—one pathway is required for efficient lambda replication, while the other has anti-viral properties inhibiting lambda replication. Based on our data, it appears that 2-thiouridine modification of tRNAGlu, tRNAGln, and tRNALys is particularly important for the efficient production of infectious lambda phage particles.

Author Summary

In this study, we took advantage of a new genetic resource for E. coli mutants to screen for previously undiscovered lambda phage host-dependencies. We then assessed the dynamics of infection in these different E. coli mutants and applied a mathematical model of infection in an attempt to further classify the role of these novel interactions. This model-driven approach to biological discovery led us to identify the previously uncharacterized gene yneJ as a regulator of lamB gene expression. In addition, we identified two highly conserved pathways involved in post-transcriptional modification of tRNA—one pathway was required for efficient lambda replication, while the other has anti-viral properties inhibiting lambda replication. This finding is important as it illustrates a new potential anti-viral strategy that could be applied broadly to other viruses.

Introduction

Viral infections present a deadly paradox: in spite of the apparent simplicity of the viral genome, the complexity of the infection process has, for the most part, thwarted our attempts to prevent or cure it. Viral infections pose a serious threat to populations in both developing and developed countries. Additionally, viral infection is a serious problem for the bioprocessing industry, threatening production of items ranging from food to pharmaceuticals [1]. Increasing our understanding of viral infection would therefore have a major impact on human health, industry, and quality of life.

One resolution of this paradox is that the complexity of infection is not limited by the scope of the viral genome, but by the host machinery that the virus must commandeer in order to replicate. Recently, several genome-scale experimental studies have sought to identify these host-dependencies in viral replication. Research groups studying HIV [2][4], Influenza virus [5], [6], West Nile virus [7], Hepatitis C [8], [9], yeast virus [10], and T7 bacteriophage [11] have made use of newly constructed host knockout or siRNA knockdown libraries, in order to perturb the host and identify host dependencies. These forward-genetic screens have identified hundreds of host factors involved in viral infection and have provided a greater appreciation for the host's contribution to viral infection.

Today, the best-characterized model of viral infection remains bacteriophage lambda and its host—E. coli. Lambda is a temperate phage with two possible outcomes upon cell entry. In lytic growth (also known as productive growth), phage quickly replicate and lyse the cell, releasing new phage particles into the surrounding environment. In lysogenic growth, the injected phage DNA integrates into the attB site of E. coli genome and becomes a prophage [12]. The inserted prophage lies dormant until a later time, when upon induction the prophage genome excises itself from the host genome and begins productive growth. The determinants of lytic versus lysogenic growth appear to depend on several factors, such as multiplicity of infection [13], temperature [14], [15], and host cell physiology (e.g., nutrient state and size) [16], [17]. The lambda-E. coli system has also been a central player in elucidating and helping to understand host-virus interactions. Many genetic screens have been used to understand the infection phenotypes of different virus and host mutants [18]. These studies have greatly increased our knowledge pertaining to viral infection.

In this study, we focused on determining the interactions between E. coli and lambda phage during the infection process. We began with a forward-genetic screen to identify the E. coli genes whose absence results in a significantly reduced infection by phage lambda. We then performed higher resolution measurements of the infection time course for each gene and used a combination of bioinformatics and mathematical modeling in an effort to more rapidly identify likely roles in the lambda lifecycle.

Results

Lambda infectivity screen

Our screen to determine E. coli genes involved in lambda phage infection made use of the “Keio Collection”, an in-frame single-gene knockout strain collection, which contains 3,985 strains corresponding to all the genes which are non-essential during growth in rich medium [19] (see Figure 1A). We grew each knockout strain, as well as the “wild-type” K-12 MG1655 strain (K-12 WT), together with lambda phage on an agar plate with nutrient broth (NB) and 24 hours later assessed the resulting plaque morphology. In the first pass, 152 knockout strains appeared to affect lambda replication efficiency, producing either no visible plaques or smaller plaques relative to K-12 WT. All of the strains that appeared to inhibit phage replication, along with an additional 88 strains that were difficult to assess—primarily due to lawn defects—were considered further in two replicate experiments.

Figure 1
A large-scale screen to determine the E. coli genes required for phage lambda infection.

In all, 57 strains were identified with significantly different plaque morphology from K-12 WT (see Figure 1B and Table S1). The genes corresponding to these strains fall into three categories with respect to annotation: (i) genes with a known role in lambda infection, (ii) well-characterized genes whose products had nevertheless not been implicated in lambda infection, and (iii) unannotated genes.

The first group—well-known E. coli genes involved in lambda infection—included 19 genes. These include genes involved with lambda transport including lamB, which encodes a membrane protein required for the phage to bind E. coli [20], as well as transcriptional regulators of lamB: malT [21], malI [22] and cyaA [23], [24] (see Figure 2A). The inner membrane transporter manZ is part of a mannose PTS permease that is thought to be used by lambda phage to transport its genome into the cytoplasm [25], [26]. cyaA plays a dual role in lambda infection as it regulates expression of lamB and is involved in the lysis-lysogeny decision [24], [27].

Figure 2
Schematics of E. coli pathways and networks involved in lambda infection.

In addition to cyaA, other genes involved in the lysis-lysogeny switch were found, including the proteases encoded by hflC, hflK and hflD. The FtsH-HflKC complex contributes to E. coli lysis by degrading the cII lambda transcription factor [28]. HflD directly interacts with cII, facilitating its degradation as well as disrupting its DNA binding ability [29], [30]. ihfA and ihfB were also found in the screen, and their gene products form a complex called integration host factor (IHF), which has been shown to induce sharp bends in DNA and is required for the integration of the prophage into the E. coli genome [31]. IHF has also been shown to play a role in phage DNA maturation [32].

The chaperone DnaJ contributes to a complex that works to destabilize the lambda P-DnaB complex bound to the ori site, thus allowing the DNA to be unwound and replicated [33]. The antiterminator gene nusB is known to play an important role in transcriptional dynamics of phage infection [34].

gmhA, gmhB, hldD, hldE, rfaC, rfaF, rfaH, and rfaP are all involved in the synthesis of the inner core of lippopolysaccharide (LPS) and were shown to affect the ability of phage to infect each strain (see Figure 2B). ADP-L-glycero-ß-D-manno-heptose is a key precursor to the inner core of LPS and is synthesized from D-sedoheptulose-7-phosphate by the gene products of gmhA, gmhB, hldD, and hldE. The heptose is then covalently bound to the KDO-Lipid A region by rfaC. All of the genes in the pathway, up to and including rfaP (with the exception of rfaG, whose activity may be replaced by rfaJ), showed reduced infectivity in our screen. This corresponds to the point in the pathway where the first heptose is phosphorylated. These eight LPS biosynthesis genes represent ~73% of the genes found in a recent screen for E. coli genes required for T7 infection [11].

Previous work has shown that K-12 strains with varied LPS compositions have altered lambda receptor activity [35], [36]. Two possible explanations of this observation have been suggested. One study showed that mutations for LPS synthesis reduce the number of surface LamB proteins [35] while it has also been suggested that altered LPS configuration leads to non-optimal arrangement of LamB receptors, by analogy to the T4 phage receptor OmpC [36], [37]. These explanations are not mutually exclusive.

The second group of E. coli genes identified in our screen consisted of 34 genes with known functional roles but no previous link to lambda phage infection. Interestingly, the largest functional category in this group appears to be metabolic. Several of the identified genes play a role in central metabolism, including several key enzymes (pgi, pgm, atpA, talB, fucA), transporters (crr, lamB, manZ), and regulators (cyaA, malT, malI, fruR, bglG, see Figure 2C). Furthermore, the glucokinase encoded by glk was not included in our initial list but likely inhibits lambda replication as only one relatively small plaque was observed in our screen.

iscS, tusA, tusE, and mnmA were all found in our initial screen and are involved in the thiolation of tRNA [38]. iscS is necessary for thiolation of all nucleosides while tusA, tusE, and mnmA gene products contribute specifically to 5-(carboxy)-methylaminomethyl-2-thiouridine modification of tRNAGlu, tRNAGln, and tRNALys.

Several other interesting genes emerged in the second group. spr is an outer membrane lipoprotein, which for certain mutants, show thermosensitivity [39]. Intriguingly, mutants of nlpI, also found in our screen, have been shown to suppress this sensitivity [40]. pepA expresses aminopetidase A/I, which is involved in gene regulation, maintaining plasmid monomers, and preventing plasmid trans-recombination [41]. RlmE is the methyltransferase responsible for methylating U2552 of 23S rRNA [42]. Mutants for rlmE show reduced growth rate, protein synthesis activity, [43] and can modulate translational accuracy [44].

Four genes found using the screen are essentially uncharacterized. The structure of YbeD has been determined and may play a role in lipoic acid biosynthesis or the glycine cleavage system [45]. Global bioinformatic analysis revealed that YneJ has a LysR-type DNA binding domain and may therefore be a transcription regulator [46]. YfiM might act as an ABC transporter [47] and yecR has appeared in a computational screen to identify genes regulated by the flagellar master regulator FlhD2C2 [48].

Infection dynamics of E. coli strains showing reduced infectivity

We wondered how best to characterize the functional roles of new genes implicated in lambda infection. One weakness of the previous screens for host gene requirements in viral infection is that the information produced by these screening experiments is highly limited, generally involving only a few measurements per gene.

We hypothesized that higher time-resolution monitoring of infection dynamics would facilitate validation and further characterization of the roles these host genes play in the lambda phage lifecycle. We monitored E. coli growth and lysis over a full course of lambda infection in liquid culture (see Figure 3A). Infected K-12 WT bacteria grow exponentially for about 3 hours, after which the rate of bacterial lysis briefly outpaces growth. During this time, many phage have also induced lysogeny in their E. coli hosts, which then become resistant to further lytic infection. The lysogenic strains eventually take over the culture, growing exponentially until stationary phase.

Figure 3
E. coli growth curves under normal conditions and incubated with lambda phage.

We monitored growth of infected and uninfected cultures for all 57 strains that showed reduced infectivity in our plaque assay. We found that the infection dynamics varied significantly between strains. Figure 3B shows selected time course data, normalized by growth rate and maximum carrying capacity (i.e., optical density at stationary phase) to highlight the difference between infected and uninfected strains (The infection time courses for all 57 strains can be found in Figure S1).

We observed that genes with directly cooperative roles in lambda infection often exhibited very similar growth and clearance dynamics. As a simple example, Figure 3C shows the infection time courses for ΔlamB, ΔmalI, and ΔmalT. As mentioned above, all of these genes work together—malT and malI regulate the expression of the lamB transcript and functional protein product.

Clustering of infection dynamics

This observation suggested that similar infection time courses between knockout strains might be an indicator that the corresponding gene products act together in a pathway required for lambda infection. We performed agglomerative hierarchical clustering on the processed time course data to help identify knockout stains with similar infection dynamics (see Figure 4). To reduce the effects of varying growth rate between strains and to focus on the key transitions in the infection time courses, we pre-processed our data to obtain a normalized time course of the infection curve derivative for each strain (see Materials and Methods).

Figure 4
Clustered E. coli growth curves under infection conditions for all of the reduced infectivity strains.

In all, we identified 18 separate clusters, separated primarily by: (i) the time point at which cell lysis outpaced cell growth, (ii) the length of time to achieve maximum clearance, and (iii) the re-growth or lysogenic growth rate. As an example, Clusters 17 and 18 show similar dynamics for properties (i) and (ii), but Cluster 17 shows limited secondary/lysogen growth. Genes in clusters with limited secondary growth are particularly interesting because they may play a role in lysogenization, as exemplified by Cluster 9, which contains hflC and hflK—two known regulators of lysogenization. However, this interpretation comes with the caveat that the secondary growth occurs under slightly different nutrient conditions than the primary growth phase.

Two major clusters bookended the dataset. At one end, Cluster 18, which was largely comprised of K-12 WT samples, showed rapid growth and lysis followed by robust secondary growth. Interestingly, two genes, yfiM and rutE, which were identified in our initial screen and consistently showed small plaques in the plaque assay, clustered with this group.

The largest cluster, Cluster 3, falls at the opposite end of the spectrum from the K-12 WT cluster and is characterized by little or no lysis over the entire time course. This cluster includes many of the previously known E. coli genes whose absence prevents lambda infection, such as lamB. There is a strong correlation between the plaque assay and infection time course as eight (ΔdnaJ, ΔyneJ, ΔmalI, ΔmalT, ΔlamB, ΔmanZ, ΔrfaF, and ΔrfaC) of the nine strains that had zero plaques in all trials fell into this cluster (see Table S1). The one exception corresponds to the outer membrane lipoprotein named spr (Cluster 15). Of the remaining genes in this cluster, Δtpx, ΔihfB, ΔgmhA, and ΔhdlD showed zero plaques in the initial screen and small plaques in the validation plaque assays. The two remaining genes in this cluster, Δcrr and ΔihfA, produced small plaques in each plaque assay and very little clearance in the liquid culture assay.

Several other genes involved in the same biological pathway were also found in the same cluster, for example, hflC and hflK (Cluster 10); lamB, malT, and malI (Cluster 3); and many of the LPS pathway genes (Cluster 3). Interestingly, pgi and talB (Clusters 14 and 15) both catalyze formation of fructose-6-phosphate and demonstrate similar infection dynamics. However, some genes involved in shared pathways did not cluster together. For example, ΔpdxH and ΔpdxA showed very different dynamics and clustered at opposite ends of the clustergram.

The finding that strains from multiple pathways all exhibited similar dynamics in Cluster 3 was intriguing, and we wondered if we could further discriminate between members of this cluster. We monitored the total E. coli concentration during infection at higher (10- and 100-fold) multiplicity of infection (MOI) for each strain in the cluster (see Figure 5A and Figure S2). After normalization, we compared the difference in the population between the uninfected and infected samples (see Figure 5B). We found that the higher MOI values appeared to have no effect on several strains, including ΔlamB, ΔdnaJ, ΔmalI, ΔmalT, ΔnusB, Δtpx, and ΔyneJ. tpx and yneJ are particularly interesting as their roles in lambda phage infection are entirely unknown. Those strains that did appear to be affected by higher MOIs corresponded to the genes involved in biosynthesis of inner core LPS, ihfA, ihfB, and manZ.

Figure 5
The effect of increased phage concentration on infection dynamics.

At the higher MOIs, the genes involved in LPS synthesis appeared to separate into two groups based on peak times (see Figure 5C and 5D). With the exception of gmhB, the genes required for attaching heptose to the KDO group had nearly identical peak times. Others have shown that ΔgmhB does not produce an entirely heptoseless form of LPS and conclude that there is another phosphatase that can catalyze this reaction [49]. ΔrfaF, ΔrfaP, and ΔrfaH had peak times much closer to K-12 WT.

Computation model of infection dynamics and the characterization of yneJ

We found the identification of unannotated gene yneJ to be of particular interest. Infected ΔyneJ showed no visible plaques and growth dynamics nearly identical to uninfected samples. We decided to apply mathematical modeling to interpret our infection time courses and help direct our efforts in characterizing the role of yneJ in lambda phage replication.

The population level interaction of phage with bacterial hosts has previously been phrased as a predator-prey system of differential equations [50], [51]. Following these previous efforts, we constructed a model that defines three populations as concentrations: uninfected bacteria, lysogens, and infectious phage (see Figure 6A). We then considered the effects of three key parameters on infection dynamics: (i) the burst size b, meaning the average number of infectious phage released upon host cell lysis, (ii) the fraction f of infection events that proceed down the lytic pathway, and (iii) the rate ki at which infection occurs. We found that we could recapitulate the infection time courses we observed simply by varying the parameters in our model (see Figure 6B, compare to Figure 3B).

Figure 6
Numerical simulations of E. coli growth during phage lambda infection.

To determine how model parameters could create different phenotypes, we simulated an infection time course for five levels of each of these three key parameters (125 simulations in total). The parameter combinations led to simulations that strongly resemble virtually all of the experimental time courses we observed (see Figure S3). We clustered the derivatives of the simulated time courses and found that the variation between simulations likewise resembled the variation between experimental strains (see Figure 6C and Figure S4). The one significant exception to this observation was that many of the simulations actually led to enhanced phage infection.

Importantly, the same types of variation that were found in the experimental time course cluster were also found in the simulated data cluster. We therefore wanted to determine which parameter combinations contributed to which type of variation. We found that the variation in f primarily contributes to the re-growth of the lysogenic population (see Figure 6C, right). In contrast, there is some correlation between b and ki (see Materials and Methods), but we found that the product b*ki varies inversely with the time at which lysis outpaces cell growth (see Figure 6C, far right).

This relationship between the parameters b and ki undermines the hypothesis that strains with a similar infection time course are involved in the same pathway, because multiple parameter combinations can lead to identical time courses. For example, the no-infection phenotype exhibited by members of the lamB cluster can be created computationally by setting f, b, or ki to very low values (see Figure 7A for the simulations and Figure 3C for representative data). However, the computational scenarios that produce equivalent total E. coli concentration time courses (see Figure 7A) create significantly more variation in the lambda phage concentration time courses (see Figure 7B). Specifically, the situation when lambda cannot infect the host at all (equivalent to setting ki to zero) leads to a stable concentration of phage over time, and when no viable phage are produced by infection (a low or zero value for b), the phage concentration is steadily reduced over time. In the third scenario, viable phage is produced at a rate exceeding its absorption (initially) and thus accumulates, however rate of production is very low (low f, ki, or b) and insufficient to produce host lysis on an observable scale. Accumulated phage populations in the latter case are orders of magnitude lower than observed for wild type.

Figure 7
The use of phage production time courses to further discriminate between strains with similar E. coli infection curves.

To test these model predictions, we compared them to phage concentration time courses that we generated for members of the lamB cluster (see Figure 7C). We found that the simulated time courses compared favorably to our experimental data, in that infection of the lamB strain led to a nearly constant phage concentration, as would be expected if phage coul;d not infect the host. We also found that infection of the dnaJ strain, which is necessary for replication of lambda DNA, led to a decrease in phage concentration. In contrast, the ΔmanZ, ΔmalI, and ΔyneJ strains all produced significant amounts of phage over time, albeit less than the K-12 WT.

Our results of the phage concentration time courses suggest that the effect of ΔyneJ on lambda infection is within the low f, ki, or b range. To investigate if the loss of yneJ might affect the lytic-lysogenic decision (f) or the relative infection rate (ki), we performed single cell analysis of K-12 WT and ΔyneJ cultures infected by GFP-expressing lambda phage (see Figure 8A). We observed a large decrease in the percentage of ΔyneJ cells initially infected relative to K-12 WT (see Figure 8B), while lysis occurred at approximately the same time relative to K-12 WT. In addition, K-12 WT demonstrated a very low frequency of lysogeny, where only 2 of 27 infected cells appeared to become lysogens. We did not observe any lysogens among the 10 infected ΔyneJ cells. Based on these results, it does not appear that the reduced infectivity of lambda phage in ΔyneJ is due to a high frequency of lysogens (low f), but more likely, a reduced infection rate (low ki). This is consistent with ΔyneJ showing similar dynamics to other knockouts that are known to affect infection rate (i.e., ΔmanZ, ΔmalI, and ΔmalT) for both the infection and phage concentration time courses.

Figure 8
Determining the function of yneJ.

We hypothesized that similar to MalI and MalT, YneJ might play a role in the regulation of lamB. To test this hypothesis we used quantitative real-time RT-PCR to examine lamB mRNA expression in K-12 WT, ΔlamB, ΔmalT, ΔmalI, and ΔyneJ cultures. We found that ΔyneJ had a significantly reduced expression of lamB (see Figure 8C). lamB mRNA levels in ΔyneJ were comparable to levels found in ΔmalI mutants.

U34 tRNA thiolation and lambda infectivity

Sulfur used for the thiolation of tRNA nucleosides in E. coli is first transferred to IscS. Depending on the tRNA and the particular base modification there are two distinct pathway classes: an iron-sulfur ([Fe-S]) protein-independent and a [Fe-S] protein-dependent pathway [52]. Our plaque assay results found several genes in the [Fe-S] independent pathway responsible for thiolation of U34 for tRNAGlu, tRNAGln, and tRNALys. In this pathway, sulfur is transferred from IscS to TusA. TusB, TusC, and TusD form a heterotrimer complex where Cys78 of TusD is able to form persulfide, facilitating transfer of sulfur from TusA to TusE [38]. Sulfur is then passed from TusE to MnmA, which thiolates uridine 34 of the tRNA. Our plaque assay screen showed reduced infectivity for all strains in this pathway with the exception of ΔtusB, ΔtusC, and ΔtusD. For ΔtusB, ΔtusC, and ΔtusD, we do observe a slight reduction in efficiency of plating and the plaques are generally smaller then the K-12 WT controls (data not shown).

In the [Fe-S] dependent pathway, sulfur is transferred from IscS to IscU. This transfer is facilitated by several proteins, including IscA, Fdx, and the chaperone/co-chaperone pair HscA and HscB. As it is thought that IscU binds to IscS, potentially competing with TusA for sulfur, we looked more closely at the proteins in the [Fe-S] dependent pathway. We found that ΔiscU, ΔhscA, and ΔhscB showed significantly larger plaques compared to K-12 WT (data not shown).

In addition to the four tRNA genes identified in the original screen, we examined the infection dynamics for ΔtusB, ΔtusC, ΔtusD, ΔiscU, ΔhscA, ΔhscB and a ΔtusBCD strain (see Figure 9 and Figure S5). The ΔtusB, ΔtusC, and ΔtusD strain infection dynamics were indicative of reduced infectivity, showing a significant delay in the peak. ΔtusBCD had very similar dynamics to the individual knockouts for tusB, tusC, and tusD. The infection dynamics for ΔiscU, ΔhscA, and ΔhscB cleared relatively quickly and had very little secondary growth.

Figure 9
Pathways involved in sulfur metabolism and the thiolation of tRNA nucleosides affect lambda replication both positively and negatively.

Discussion

In summary, to determine the E. coli gene requirements for lambda infection, we performed a screen of 3,985 non-essential gene knockout strains and found 57 strains with impaired lambda infectivity. In addition to identifying many genes with established roles in lambda phage infection, we found a surprising number of previously unassociated genes, four of which are currently unannotated. In addition, several of the genes found in our screen have human orthologues (see Table S2).

Central metabolism was the largest shared functional category among our results. In particular, we found many genes involved in multiple entry points to and regulators of glycolysis. This observation is in part related to lambda phage's dependence on LamB and the factors that regulate lamB expression. Several other metabolic genes identified in our screen are known to play a role in regulating the lytic-lysogenic decision. Based on this observation, it is tempting to speculate that many of these genes may influence lysogeny, whether by sensing or altering the cell's nutritional state. Our results potentially expand this lytic-lysogenic network and provide a framework for a deeper understanding of this decision as well as the metabolic requirements for lambda phage replication. It is interesting to note that many of the host-dependencies identified in the recent mammalian virus screens are also involved in energy metabolism and enzymes involved in amino acid and nucleic acid synthesis.

Second, we demonstrated that the knockout strains for genes with common roles in infection often showed similar infection dynamics. Some examples include the hfl, ihf, LPS biosynthesis and lamB-related genes. Our observation is complicated by at least three factors. One complication arises when the effect of gene deletion within a pathway varies depending on the step within the pathway, as in the LPS biosynthesis pathway. Another confounding factor is that some proteins may be partially redundant, where in the absence of one protein another can adequately compensate thus producing a mild or no change in phenotype. This may be the case for GmhB and an unidentified phosphatase. While we did not identify the complementary phosphatase in this study, one might look among the strains clustering with ΔgmhB. Finally, many proteins have pleiotropic effects and the observed dynamics may arise from the modulation of multiple pathways. An example of this is the protein CyaA, which has a metabolic function but also plays a role in the lytic-lysogenic decision. Notwithstanding these exceptions, dynamic infection data was extremely useful as a validation tool and a “first-step” in assessing host gene functionality in lambda infection.

We used a combination of computational modeling and further experimentation to characterize many of the strains in more detail. This was best exemplified by our efforts to characterize the previously unannotated gene, yneJ, and its apparent critical role in infection. We observed that ΔyneJ closely resembled the ΔmanZ, ΔmalT, and ΔmalI strains in terms of growth phenotype, lambda phage production, and response to higher phage concentration. Using single-cell imaging of GFP expressing lambda phage, we found that ΔyneJ is not immune to infection and does not appear to regulate the lytic-lysogenic decision. We suspected that yneJ may play a role in attachment or entry, possibly through the regulation of LamB or another unidentified membrane-associated protein and tested the expression levels of lamB in several strains including ΔyneJ. Our data demonstrated a reduced level of lamB mRNA in ΔyneJ similar in magnitude to ΔmalI. Given YneJ's LysR-type DNA binding domain, we speculate that YneJ is an upstream regulator of lamB transcription—possibly directly or indirectly regulating malI expression. Given its effect, it is intriguing that yneJ was not identified over the several decades of reverse-genetic screening of phage lambda.

Another surprising result of this work was the identification of two important pathways for lambda phage replication with a common node at cysteine desulferase IscS. Interestingly, inactivation of one of these pathways (including tusA, tusB, tusC, tusD, tusE, and mnmA) leads to impaired lambda infection, while inactivation of the other pathway (including iscU, hscA, and hscB) facilitates lambda infection.

Others have shown that the 5-(carboxy)-methylaminomethyl-2-thiouridine modification at the tRNA wobble position increases frame maintenance and prevents codon-specific frameshift in E. coli [53]. We hypothesize that the rapid and proper synthesis of lambda phage proteins is particularly dependant on this modified nucleoside. Viruses of infected cells lacking this modification likely show decreased production of functional viral proteins and thus produce a smaller number of infectious particles. In concept, this hypothesis resembles the lethal mutagenesis therapeutic strategy for treating viral infection [54], albeit at the protein level. Based on our data, it appears that 2-thiouridine modifications of tRNAGlu, tRNAGln and tRNALys are particularly important for the efficient production of infectious lambda phage particles. The s2U34 modification is conserved for several tRNAs across all organisms [55], raising the question of whether these genes or related pathways might present novel anti-viral targets for mammalian viruses.

Materials and Methods

“Keio Collection” screen

Our screen was performed using the established plaque assay method [56]. K-12 WT (ATCC, 47076) and all strains of the “Keio Collection” were cultured overnight (~16 hours) in nutrient broth (NB, 8 g/L, Fluka Analytical, N7519) using 96 deep-well plates (Nunc, #278743). Incubation was done at 37°C while rotating at 225 RPM. Each E. coli strain was incubated with bacteriophage lambda (ATCC, 23724-B2) for 30 minutes at 37°C—optimal titers for bacteriophage lambda were determined beforehand using a dilution series. 2% 2,3,5-Triphenyltetra-zolium chloride (Sigma, T8877) was added to NB top agar (0.04% final concentration) and incubated at 55°C for 30 minutes. The top agar was then added to the incubating E. coli and phage samples and 80 µl was plated onto 24-well agar plates. The agar plates were made the previous day with 500 µl of NB bottom agar for each well. Included on each plate were two replicates of infected K-12 WT and one well of ΔlamB. After 24 hours, the number of plaques generated by infection of each strain was counted and compared to K-12 WT counts. Wells with significantly fewer or smaller plaques for two replicate experiments were considered “hits”.

Infection time courses

To monitor the E. coli concentration of an infected batch culture over time, we used an incubated plate reader (Perkin-Elmer Victor3, 2030-0030). Strains of the “Keio Collection” were inoculated and grown overnight (~16 hours) in 2 ml NB in 5 ml round-bottom tubes. The next morning the samples were diluted 1[ratio]100 in fresh NB media and grown for 3 hours. After 3 hours the samples were measured for absorbance at 600 nm and diluted in NB to 0.1 OD. 15 µl of 0.1 OD E. coli and 15 µl of ~104 plaque forming units/ml (pfu/ml) lambda stock were added to 170 µl of NB in 96-well plates—representing an MOI of ~2×10−4 pfu/bacteria. Four replicates for each low infectivity strain (infected and uninfected) were assayed. Strains ΔatpA, ΔthyA, and ΔiscS did not show significant growth rates over the time course, and therefore provided no additional information concerning phage infection. The “Keio Collection” was created using E. coli BW25113 as the background strain, so we compared the infection dynamics of this strain with E. coli MG1655 and found them to be essentially identical (see Figure S6).

Included on each plate were replicates of K-12 WT. The incubation protocol included an initial 10 minute shake (double orbital, 1.5 mm diameter, normal speed), followed by 38 cycles consisting of the following actions: a one second absorbance measurement at 600nm (Perkin Elmer, 600/8nm, 1420-521), 5 µl injection of milliQ water into each well (to counter volume loss due to evaporation), and a 10 minute shake (double orbital, 1.5 mm diameter, normal speed). The time course was performed at 37°C for approximately eleven hours.

Lambda phage time course quantification

The K-12 WT, ΔlamB, ΔmanZ, ΔmalT, ΔmalI, ΔdnaJ, and ΔyneJ strains were inoculated in NB and grown overnight at 37°C while rotating at 225 RPM. The next morning the samples were diluted 1[ratio]100 in fresh NB media and grown for 3 hours. After 3 hours the samples were measured for absorbance at 600 nm and diluted in NB to 0.1 OD600. 375 µl of E. coli, 375 µl phage stock, and 4.25 ml of NB at 37°C were combined in 14 ml tubes. Aliquots were taken from each culture at 90, 173, 205, 236, 276, 322, 364, and 415 minutes post-infection and filtered using 0.2 µm PES filters (Nalgene, 180-1320). The filtrate was then diluted in SM + gelatin (0.058% (w/v) NaCl, 0.02% (w/v) MgSO4-7H2O, 50 mM Tris (pH 7.5), 0.01% gelatin). 100 µl of these dilutions were incubated with an equal quantity 2.0 OD600 E. coli in 10 mM MgSO4 for 10 minutes before combining with 1 ml NB top agar 500 µl onto 6-well plates. After incubating overnight, the plaques were counted to determine the pfu/ml at each time point.

Infection time course data processing

A key challenge in our data processing was to determine a metric to compare two infection time courses. Observing that uninfected knockout strain time courses cluster by pathway based solely on the variation in background growth phenotype, normalization of infected growth curves was necessary in order to avoid clustering these based on the similar behavior of their bounding uninfected curves. To prevent clustering based on growth rate and the eventual population limit, we non-dimensionalized the growth time courses for each strain using parameters of logistic population growth fit to uninfected data (model presented, simulated as uninfected using initial condition [λ] = 0 at t = 0). The carrying capacity, K, was considered the characteristic population and inverse growth rate 1/μ the characteristic time. This treatment allowed us to compare the key features of the infected time courses relative to their background, for example allowing distinction between a strain that is overtaken by phage late due to generally weak/slower growth/metabolic function and one that is overtaken late despite quick/normal growth potentially indicating a more phage specific knockout impact. Although deemed necessary for the meaningful data interpretation via our method, anytime rescaling is performed to clarify certain dataset features, the potential exists to deemphasize or obscure other features of that data set, and we have thus presented our entire raw dataset in Figure S1. Data was smoothed using the robust lowess implementation in MatLab (window size 0.1 as a fraction of total data points), followed by analytical calculation of the time derivative from a cubic smoothing spline to avoid noise amplification. A cosine distance metric was used in clustering, 1-θ, where theta is the included angle between time course derivatives treated as vectors, emphasizing similarities in population change direction rather than magnitude. Agglomerative hierarchical cluster tree was constructed with average linkage, and clusters defined by a linkage of less than 0.16.

Computational modeling of lambda phage infection dynamics

We constructed a model that defines three populations as concentrations: uninfected bacteria [E], lysogenically-infected bacteria [E*], and infectious phage [λ]. Bacterial growth is assumed to occur logistically with rate μ towards a limiting population [K]. We used analogous but separate parameters for lysogens (denoted by *) [57].

The ordinary differential equations are as follows:

equation image

Mass-action kinetic infection of bacteria by phage, with rate ki, is well established [58]. Superinfection of lysogens occurs with no effect other than to reduce the infection phage population [59]. The amplification factor parameter b represents the average number of infectious phage released upon host cell lysis. Lysogen induction to the lytic pathway by DNA damaging stresses is included at rate ks for the sake of completeness, but is assumed negligible under our conditions and henceforth neglected. f is the fraction of infection events that proceed down the lytic pathway. Given the complex nature of the lambda decision and switch (and neglect of ks), f as a constant fraction is necessarily an average parameter containing information on the ease of lysogeny establishment and maintenance.

For the purposes of well-scaled numerical simulation the model was converted to a non-dimensional form using the same characteristic time and population as for the experimental time courses. Replacing the time with its product with μ, and dividing each population variable by K, both maximum growth rate and maximum population reduce to unity. The parameters f and b are retained as fraction and amplification factor respectively, while lysogen growth reduce to ratios to their analogous uninfected growth parameters, and ki becomes the dimensionless group kiK/μ. All simulations presented were completed using the scaled form, and values of parameters listed are the corresponding non-dimensional form or group.

All numerical integration was completed using the standard MatLab implementation of rk45, with default tolerances. The initial condition [E]t = 0 = 0.02 was chosen and used for all simulations based on values fit simultaneously as logistic kinetics were fit to experimental data (least squares distance), with [λ]t = 0 set using the experimentally determined MOI, and no initial lysogen population ([E*]t = 0 = 0). The simulation results for the E. coli population presented are the sum [E]+[E*], as these populations are not distinguished experimentally during our infection time course observation. Simulations were clustered using the same method as experimental data (though smoothing was unnecessary). Parameter values used in the simulations, displayed in Figure S3 and Figure S4, were all possible combinations of ki = {0, 0.25, 0.75, 2, 5}, f = {0, 0.5, 0.75, 0.95, 1}, b = {0, 10, 20, 50, 100}. Values for f and b were chosen as physically reasonable values. The set of values for ki were then chosen from the range that produced model behavior resembling our experimental observations. It should be noted that for a given infection time course simulation, a practically equivalent bacterial population time course can be generated using alternate combinations of the parameter ki and b values. The lysogen growth character was not varied, using constant μ* = K* = 0.7 for all simulations, both because our primary focus was on the character of the infection process that leads to the initial overtake of the bacterial population by phage, and also because at later times in batch culture it is possible that our experimental observations of lysogen growth character are dominated by nutrient limitation.

Single-cell imaging of GFP–expressing phage infection

Exponentially growing cells were infected with lambda b::GFP kanR [17]. Adsorption of lambda (MOI≈0.5) was done at 4°C for approximately 20 minutes. 1 µl of sample was pipetted onto a 2% agarose pad. The agarose pad was made using equal volumes of 4% LMP agarose and 2× EZ-RDM (Tecknova, M2105) supplemented with 2% maltose, 20 mM MgSO4, and 1mM of IPTG to induce expression of the GFP construct. The pad was then inverted onto a cover slide and a plastic lid was placed on top to help prevent drying of the pad over the time course. The assembled slide was maintained at 37C during imaging. Both phase (30 ms) and GFP (50 ms) images were taken every 2 minutes at 60× magnification. Cells were manually assessed for infection.

Quantitative real-time RT–PCR of lamB

Exponentially growing cells were treated with RNALater (Ambion, AM7020) according to the manufacturer's recommendations. The RNA was then isolated using Qiagen's RNeasy Mini Extraction kit (Qiagen, 74104). DNase digestion was performed on the RNA sample using Deoxyribonuclease I (Invitrogen, 18068-015). First-strand cDNA synthesis was performed (Invitrogen, 18080-051) followed by RNase H digestion. 100 ng of template cDNA and primers (200 nM final concentration) were combined with the SYBR Green PCR master mix (Applied Biosystems, 4367659). LamB (left primer, 5′- ATGAGCACCGTGATGGAAAT -3′; right primer 5′- AGCGTTACCGGTGTAGTCGT -3′) and rrsA (left primer, 5′- CGGTGGAGCATGTGGTTTAA -3′; right primer, 5′- GAAAACTTCCGTGGATGTCAAGA -3′) primers were run in quadruplicate for each strain. K-12 WT cDNA dilutions (2×, 4×, 10×, and 100×) were used to calculate the primer amplification efficiency.

tusBCD knockout construction

The ΔtusBCD strain was constructed according to methods described elsewhere [60]. Primers were designed to knockout all 3 genes as one continuous fragment and replace it with the chloramphenicol acetyl transferase gene from pKD3. The upstream primer was 5′-TACATCCGCCAGTTCAAGAGCGGTGATTTCCAGGGGCAAGATAAGTAATGATGGGAATTAGCCATGGTCC-3′ and the downstream primer used was 5′-GTGTCAAGAAATATACAACGATCCCGCCATCACCAGGCCATCTGGCTGGGGTGTAGGCTGGAGCTGCTTCG-3′.

Supporting Information

Figure S1

The raw E. coli growth time courses for the wild type strain and all of the knockout screens with lower-than-wild type infectivity. The gene missing from the strain is shown in the upper left corner of each graph. To facilitate comparison between strains cultured on the same plate, the plate number is indicated by the subscript (e.g., the ΔyfiM strain was cultured in Plate 6, and can be compared to the K-12 WT strain that was also cultured on this plate).

(1.25 MB PDF)

Figure S2

E. coli growth time courses for the K-12 WT strain and the knockout strains in Clusters 2–3 (except cyaA and crr) at three MOIs. These time courses have been non-dimensionalized with respect to growth rate and maximum growth capacity (as described in the main text) to facilitate comparison between the strains.

(0.42 MB PDF)

Figure S3

One hundred and twenty five simulated infection time courses using the computational model described in the main text. The parameter values for each time course can be determined from the legends (ki and b) and trace color (f). Additional parameter values were held constant at ks = 0, μ* = K* = 0.7. These simulations have been non-dimensionalized with respect to growth rate and maximum growth capacity (as described in the main text) to facilitate comparison between the overall simulation behaviors.

(0.63 MB PDF)

Figure S4

The complete set of clustered simulation time course derivatives. Parameter values for simulations are those used in Figure S3 (for additional details see Methods and main text).

(0.51 MB PDF)

Figure S5

ΔtusBCD infection dynamics. (A) Shows the infection dynamics of the [Fe-S] independent pathway strains along with three colonies from the ΔtusBCD construction. (B) 1 - Euclidian distance between time courses for knockouts in (A) are displayed.

(0.20 MB PDF)

Figure S6

Comparison of E. coli K-12 MG1655 with “Keio Collection” background strain BW25113. Solid lines indicate lambda phage infected samples. Dash lines indicate uninfected samples.

(0.11 MB PDF)

Table S1

Plaque assay results. Irregular lawn (il), small plaques (s), and zero plaques (0) are indicated for each strain.

(0.41 MB PDF)

Table S2

Human orthologues of lambda phage host-dependency genes.

(0.31 MB PDF)

Acknowledgments

We thank Drew Endy, Karla Kirkegaard, Lynn Thomason, and Don Court for useful feedback and Francois St-Pierre, Lance Martin, Elissa Denny, and Timothy Lee for technical assistance.

Footnotes

The authors have declared that no competing interests exist.

This project was funded by a Stanford Dean's Fellowship to NDM, a Stanford Bio-X Fellowship to EWB and JCS, NSF Graduate Student Fellowships to JCS and LC, and an NIH Director's Pioneer Award (1DP1OD006413) to MWC. The funders had no role in study design, data collection and analysis, decision to publish, or preparation of the manuscript.

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