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Genetic bottlenecks facilitate the fixation and extinction of variants in populations, and viral populations are no exception to this theory. To examine the existence of genetic bottlenecks in cell-to-cell movement of plant RNA viruses, we prepared constructs for Soil-borne wheat mosaic virus RNA2 vectors carrying two different fluorescent proteins, yellow fluorescent protein (YFP) and cyan fluorescent protein (CFP). Coinoculation of host plant leaves with the two RNA2 vectors and the wild-type RNA1 showed separation of the two vector RNA2s, mostly within seven to nine cell-to-cell movements from individual initially coinfected cells. Our statistical analysis showed that the number of viral RNA genomes establishing infection in adjacent cells after the first cell-to-cell movement from an initially infected cell was 5.97 ± 0.22 on average and 5.02 ± 0.29 after the second cell-to-cell movement. These results indicate that plant RNA viruses may generally face narrow genetic bottlenecks in every cell-to-cell movement. Furthermore, our model suggests that, rather than suffering from fitness losses caused by the bottlenecks, the plant RNA viruses are utilizing the repeated genetic bottlenecks as an essential element of rapid selection of their adaptive variants in trans-acting genes or elements to respond to host shifting and changes in the growth conditions of the hosts.
Plant RNA viruses change their genomes so rapidly that variant viruses with altered biological properties are often found after prolonged growth of infected plants or after serial mechanical inoculations (26, 33). Furthermore, inoculation of less-fit artificial mutants produces revertants or pseudo-revertants even after short infection times (12, 14). The rapid evolution of plant RNA viral genomes is achieved not only by high mutation rates due to error-prone replication by the nonproofreading viral RNA-dependent RNA polymerase (19) but also by rapid selection and strong genetic drift. Generally, narrow genetic bottlenecks facilitate the fixation and extinction of variants in populations (15), and viral populations are no exception to this theory.
Plant RNA viruses are known to face many narrow genetic bottlenecks during their life cycles (23). The life cycles of most plant RNA viruses are as follows: After replicating in cells, viruses move from cell to cell through plasmodesmata, which connect the cytoplasms of adjacent cells separated by cell walls in plant tissue. Following the establishment of infection in cells and cell-to-cell movements, the viruses expand their infected regions, spreading to the veins and moving through the vascular system and infecting the plant systemically. Some plant RNA viruses are transmitted through the seeds or via mechanical injuries, but most are transmitted from plant to plant by biological vectors such as insects, nematodes, and fungi. Previous studies have found that genetic bottlenecks occur during the transfer from lower leaves to upper leaves in systemic infections of Wheat streak mosaic virus (WSMV) (11), Tobacco mosaic virus (TMV) (24), and Cucumber mosaic virus (CMV) (18) and during the transfer from one tiller to another tiller of WSMV (11). Vector transmissions were also shown to act as genetic bottlenecks for WSMV (11), CMV (1, 3), and Potato virus Y (PVY) (20). With the exception of PVY, the typical method for detecting genetic bottlenecks has been to observe the spatial separation of closely related strains or artificial synonymous mutants inoculated as mixed populations: the narrower the genetic bottleneck, the more frequently the spatial separation should be observed. Using this idea with mathematical analyses, WSMV was estimated to infect a new tiller starting with four genomes (9), TMV was estimated to infect the upper leaves starting with 10 genomes (24), and CMV was estimated to infect a new plant starting with one to two particles after aphid transmission (3). Studies of PVY using sets of host plant cultivars with or without resistance genes and mixed strains of viruses with or without resistance-breaking abilities also estimated the number of virus particles transmitted by an aphid vector to be 0.5 to 3.2 on average (20).
However, genetic bottlenecks in cell-to-cell movement of viruses have not been well characterized, although these occurrences are likely (11) and have been expected to be important for understanding the life cycle and population dynamics of plant RNA viruses. The size of genetic bottlenecks in cell-to-cell movement can be referred to as “multiplicity of infection (MOI) in plant tissue colonization,” and only a recent study showing that the estimated MOI of TMV is between 6 and 1 to 2 (10) indicates the occurrence and the size of genetic bottlenecks in cell-to-cell movement of a plant RNA virus. In this paper, we also show the occurrence of narrow genetic bottlenecks during cell-to-cell movement of a plant RNA virus, Soil-borne wheat mosaic virus (SBWMV, type species of the genus Furovirus), by observing the spatial separation of RNA2 vectors carrying different fluorescent proteins, yellow fluorescent protein (YFP) and cyan fluorescent protein (CFP). Both of the fluorescent proteins were expressed as fusion proteins to the N-terminal nuclear localization signal (NLS) peptide from Simian virus 40 (SV40) large T antigen, which enabled us to observe and count the infected cells accurately using nuclear fluorescence. Numerical data were analyzed to estimate the size of bottlenecks. We also carried out a simulation to show that, due to the narrow genetic bottlenecks, rapid selection occurs even on trans-acting elements in plant RNA virus genomes, overcoming the negative effect of complementation among adaptive and defective genomes in each intracellular population. We discuss the possible roles of the bottlenecks in the life cycle and evolution mechanisms of plant RNA viruses.
Fully expanded leaves of Chenopodium quinoa were used for inoculation after growth at 22°C for 4 to 6 weeks after sowing. Wheat (cv. Fukuho) leaves were used for inoculation after growth at 17°C for 2 weeks after sowing. C. quinoa is a local lesion host of Soil-borne wheat mosaic virus (SBWMV) used in this study, and wheat is a natural systemic host of SBWMV.
Infectious cDNA constructs for a Japanese Tochigi strain of SBWMV (SBWMV-JT), pJS1 for RNA1 and pJS2 for RNA2, were described by Yamamiya and Shirako (35). pJS2 was used as a parental vector construct for fluorescent protein gene expression. The N-CP-RT region was replaced with fluorescent protein gene sequences. YFP-coding cDNA was prepared by introducing variations in SYFP2 (17) into a SuperGlo GFP (sgGFP) gene sequence derived from pQBI25 (TaKaRa BIO, Japan). CFP-coding cDNA was prepared by introducing variations in SCFP3A (17) into the sgGFP gene sequence. The NLS coding sequence from Simian virus 40 (SV40) large T antigen and the franking sequence (translated into MDKAELIPEPPKKKRKVEL; underlined sequence indicates NLS) were derived from the pGAD-c1 vector (13) and added upstream of each fluorescent protein coding sequence. The resulting cDNA constructs were named pJS2.NLS-YFP.p19 and pJS2.NLS-CFP.p19.
In vitro transcription of pJS1- and pJS2-derived constructs were done in the presence of a cap analog using SP6 RNA polymerase (TaKaRa BIO). For reverse transcriptase PCR (RT-PCR) analysis, template DNA was digested with DNase (Promega) prior to inoculation. Transcripts were quantified by a Qubit fluorometer (Invitrogen) and added to inoculation buffer (0.1 M NaCl, 0.1 M Tris-HCl pH 8.5) at the concentrations of 7.5 ng/μl of RNA1 and 5.0 ng/μl of RNA2s unless otherwise noted and were rubbed onto the surface of assay plant leaves using carborundum as an abrasive. Inoculated plants or leaves were rinsed with water and placed in the dark at 17°C.
YFP and CFP fluorescence was observed using a fluorescent light microscope (Olympus IX70 and IX-FLA, Japan) with NIBA and U-MCFPHQ filter sets (Olympus), respectively. The images were captured using a charge-coupled-device (CCD) camera (KEYENCE VB-7010, Japan). Photoshop Element Ver 4.0 (Adobe) was used for converting the color of CFP fluorescence images into magenta and merging with YFP fluorescence images.
Total RNA was extracted using QuickGene 800 (FUJIFILM) after grinding of the frozen leaf samples by a Mixer Mill MM300 (Qiagen). SBWMV RNA2 in total RNA or RNA2 transcripts were amplified by a PrimeScript One Step RT-PCR kit (TaKaRa BIO) using two sets of primers: TP292 (5′-AACGTGCGACGTTGAGA-3′) and TP41 (5′-CTGCTGTGTAATAGCAG-3′) for amplifying almost the entire RNA2 transcript; TP292 and TP290 (5′-CACTGTGACGATACTTA-3′) for amplifying the YFP or CFP coding region (see Fig. Fig.3A).3A). DNA fragments amplified using TP292 and TP290 were cloned into a pGEM-T TA-cloning vector (Promega) for sequencing.
The nucleotide sequences for pJS2.NLS-YFP.p19 and pJS2.NLS-CFP.p19 are available from the DNA Data Bank of Japan (DDBJ) (accession numbers AB499725 and AB499726, respectively).
Soil-borne wheat mosaic virus (SBWMV), a positive-strand plant RNA virus, has a bipartite genome consisting of two RNA molecules, RNA1 and RNA2 (27, 28). RNA1 encodes replication proteins and a movement protein (MP) for cell-to-cell movement (2). RNA2 encodes the capsid protein (CP) and two CP-containing proteins: CP-RT, produced by readthrough of a stop codon, and N-CP, initiated from an upstream CUG codon (25). RNA2 also encodes a cysteine-rich protein, p19, with RNA silencing suppressor activity (29). As CP and the two CP-containing proteins are not required for replication or cell-to-cell movement (35; M. Miyanishi and Y. Shirako, unpublished data), we replaced their open reading frames (ORFs) in the infectious cDNA clone of RNA2 (pJS2) with YFP or CFP sequences fused to N-terminal NLS sequences to prepare virus vectors for YFP or CFP expression (Fig. (Fig.1).1). The YFP and CFP genes used in this study differ by 10 nucleotides, resulting in six differing amino acids. Transcripts from these cDNA clones, named RNA2.NLS-YFP.p19 and RNA2.NLS-CFP.p19, were mixed with the wild-type RNA1 transcripts and inoculated onto Chenopodium quinoa leaves. Leaves were placed in the dark at 17°C and observed under a fluorescent microscope at appropriate time points. YFP and CFP fluorescence images were taken separately and merged after the color of CFP fluorescence images was converted to magenta (an example of preparation of merged images is shown in Fig. Fig.2A).2A). YFP and CFP proteins were confirmed to mature at similar time points by inoculating barley protoplasts with the transcripts (data not shown). Inoculation without RNA1 or inoculation of template DNA did not show any fluorescence, indicating that fluorescent protein expression requires replication of RNA2 by an RNA1-encoded viral replicase (data not shown).
At 22 hours post inoculation (hpi), most of the infected sites already consisted of several infected cells. Although some of the infected sites showed only YFP or CFP fluorescence (Fig. (Fig.2B,2B, first and second panels; Table Table1),1), most of the infected sites showed both YFP and CFP fluorescence (Fig. (Fig.2B,2B, third and fourth panels; Table Table1),1), indicating that coinfection of initial cells with both the RNA2.NLS-YFP.p19 and RNA2.NLS-CFP.p19 vector viruses occurred frequently. Increasing the concentration of RNA transcripts used for inoculation did not change the number of infected sites or the frequency of coinfection (Table (Table2).2). This result indicates that the concentration of inoculated RNA was high enough to saturate all the possible infection sites. Within coinfected sites, most of the cells showed coinfection, but some of the cells showed exclusive infection by YFP or CFP vector virus (Fig. (Fig.2B;2B; exclusively infected cells can be found in the fourth panel and are indicated by white arrows). This spatial separation between YFP and CFP vector viruses progressed corresponding to the expansion of the infected regions (Fig. (Fig.2C),2C), and at 72 hpi, most of the infected sites showed absolute separation of the YFP and CFP vector in newly infected frontier cells by 7 to 9 cell-to-cell movements (Fig. (Fig.2D).2D). The occurrence of spatial separation was also observed when wheat leaves were used as a host (Fig. (Fig.2E2E).
In order to check whether mutation causes loss of fluorescence in the above experiments, we carried out RT-PCR of RNA2 vectors. When total RNA samples extracted from C. quinoa leaves inoculated with RNA1 and RNA2.NLS-YFP.p19 at 28, 48, or 72 hpi were subjected to RT-PCR, neither the primer set for almost entire RNA2 vector (TP292 and TP41) nor that for fluorescent protein coding regions (TP292 and TP290) (Fig. (Fig.3A)3A) detected a distinct amount of cDNA products shorter than the correct size (Fig. (Fig.3B),3B), indicating that deletion mutation is not a frequent event. TA cloning and sequencing of the RT-PCR product of the 72-hpi total RNA sample using the latter primer set (TP292 and TP290) showed that, out of 23 clones, two clones had deletion mutations and eight clones had point mutations (i.e., nucleotide substitutions and single-nucleotide insertions) in the fluorescent protein coding region (Table (Table3).3). However, the frequency of point mutation was not higher than that found in the control experiments cloning the RT-PCR product of the inoculated RNA transcript or the PCR product of template DNA used for transcription (Table (Table3).3). These results indicated that the point mutations detected occurred mainly in the PCR process, but deletion mutations occurred during virus infection and caused loss of fluorescence, although the frequency of deletion mutations is less than 10% until 72 hpi. We also tested the possibility of recombination during infection, but no recombination between YFP and CFP vectors was observed in 21 clones sequenced after cloning of the RT-PCR products of total RNA samples isolated from coinoculated leaves collected at 72 hpi (data not shown).
Because an NLS was added to the fluorescent proteins, we could observe the strong nuclear fluorescence and carry out numerical analysis of the infected cells accurately using infected C. quinoa leaf samples. To describe the spatial separation of the two fluorescent protein vectors corresponding to the development of the infected regions, we defined three classes of the cells by their distance from the initially infected cells: initially infected cells (Cell-0), adjacent cells (Cell-1), and following cells (Cell-2) (Fig. (Fig.4A).4A). However, as it is difficult to tell which cell is Cell-0, Cell-1, or Cell-2 in actual observations, raw data were first collected as mixtures of two or three classes of cells, and after the data from each infected site were summed up, total cell numbers were divided into the classes by simple calculation (Table (Table1).1). Detailed calculation procedures were as follows (for schematic explanation, see Fig. S1 in the supplemental material). We assumed that the number of cells classified as Cell-1 is 8 per infected site from our observation. At 22 hpi, most of the infected sites showed 5 to 9 fluorescent cells, and these 158 sites with coinfection were regarded as Cell-0+Cell-1. The number of Cell-0 cells equals the number of the infected sites, and all the Cell-0 cells should be coinfected cells. Thus, the infection status of Cell-1 cells was estimated by subtracting the number of sites (i.e., 158) from the number of YFP+CFP cells (i.e., 945), resulting in 77 YFP-only cells, 787 YFP+CFP cells, and 82 CFP-only cells. Similarly, at 28 hpi, most of the infected sites showed 10 to 30 infected cells, and these 86 sites with coinfection were regarded as Cell-0+Cell-1+Cell-2. Cell-2 infection status was estimated by subtracting the number of the sites (i.e., 86) of Cell-0 cells from the YFP+CFP number (i.e., 1,163) and subtracting the number of the sites × 8 (i.e., 86 × 8 = 688) of Cell-1 cells from the YFP-only, YFP+CFP, or CFP-only numbers at the proportion calculated from the Cell-1 calculation result [i.e., (77 + 82)/2:787:(77 + 82)/2 = 0.084:0.832:0.084], respectively. Our calculation showed that starting from coinfected Cell-0 cells, 83.2% of Cell-1 and 61.6% of Cell-2 cells continuously showed coinfection, and others showed exclusive infection by only one of the two vector viruses (Table (Table11).
We speculated that the spatial separation occurs because only limited numbers of virus vector genomes can establish infection in newly infected cells, and this limitation should be working as a genetic bottleneck for the intracellular populations. In order to estimate the number of founder viral genomes to establish infection in adjacent cells (i.e., the size of bottlenecks), we built a model as follows. First, settlement of founder genomes was regarded as a stochastic event described by the binominal distribution between two alleles, YFP and CFP: when k genomes are extracted from the mixture of YFP and CFP vectors mixed at the ratio of r:(1−r), occupation of extracted k genomes by YFP vectors (i.e., exclusive infection by YFP vector) will be observed at the probability of rk, occupation by CFP vectors (i.e., exclusive infection by CFP vector) at (1−r)k, and mixed genomes (i.e., coinfection) at 1−rk−(1−r)k (Fig. (Fig.4B).4B). The fundamental idea was to find the most likely value for k by comparing this expected ratio with the observed ratio of exclusive infection to coinfection using the maximum-likelihood method. Second, variations in the size of bottleneck k were described by the Poisson distribution, with the mean λ0, λ1 and λ2, respectively, for establishment of infection in Cell-0, Cell-1, and Cell-2 cells (Fig. (Fig.4C).4C). Third, we assumed that infection of a single cell occurs by founder genomes from an adjacent single infected cell, not from multiple cells.
By the above model, the overall probability of coinfected sites (i.e., coinfected initial cells: Cell-0) [Pmix(site)] was described by two parameters: r0, the ratio of YFP vector in inocula, and λ0, the mean size of the bottleneck in initial cell infection, as follows:
where the probability of establishment of infection by k genomes (pk) was described by Poisson distribution as pk=. Note that k0 = 1 was included in the summation in the second line because this makes the result in the square brackets zero. The likelihood of the numbers of coinfected sites (i.e., 179) and exclusively infected sites (i.e., 24) by one of the two vectors was described by the binomial distribution
The likelihood of coinfection of adjacent cells (Cell-1 cells) is a little more complicated, because infection of Cell-1 cells is affected by the proportion of YFP and CFP vectors in each Cell-0 [i.e., r1: (1−r1)]. Defining the number of founder YFP vectors that established infections in Cell-0 as l0 and the mean size of the bottleneck for adjacent cell infection as λ1, and assuming that final proportion of YFP and CFP vectors in Cell-0 follows the initial ratio of founder YFP and CFP vector [i.e., r1: (1−r1) = l0: (k0−l0)], the overall probability of coinfection of Cell-1 [Pmix(Cell-1)] in coinfected sites was described as follows:
where . Noting the binomial formula, it was further simplified as
The likelihood of the estimated number of coinfected Cell-1 cells (i.e., 787) and the estimated number of exclusively infected Cell-1 cells by one of the two vectors (i.e., 159) was described as
Similarly, defining the mean size of the bottleneck for following-cell infection as λ2, the overall probability of coinfection of the following cells (i.e., Cell-2) in coinfected sites [Pmix(Cell-2)] was described as follows:
Using the binomial formula, Pmix(Cell-2) was reduced to
and the likelihood was described as
based on the estimated number of coinfected Cell-2 cells and the estimated number of Cell-2 cells exclusively infected by one of the two vectors.
Then, substituting 0.5 for r0, we simultaneously estimated λ0, λ1, and λ2 by maximizing the total log likelihood
Calculation was done using statistical computing software R (22), and we obtained the mean bottleneck sizes λ0 = 5.59 ± 0.40, λ1 = 5.97 ± 0.22, and λ2 = 5.02 ± 0.29 (maximum likelihood estimates ± standard errors).
These results indicate that only around 5 to 6 founder genomes establish infection in adjacent cells after cell-to-cell movement. The expected size of bottlenecks for the second cell-to-cell movement (λ2) was slightly smaller than that for first cell-to-cell movement (λ1).
The estimated bottleneck sizes were used to simulate the decrease in coinfected cells corresponding to the development of infected regions. Assuming that the mean number of viral genomes that establish infection in Cell-N (λN, N ≥ 3) equals λ2, the overall probability of coinfected cells in Cell-N [Pmix(Cell-N), N ≥ 3] in coinfected sites was simulated by recurrence relation as follows:
where Pmix(site)=179/203, r0=0.5, λ0=5.59, λ1= 5.97, and λ2=5.02. The simulation result showed that fewer than 10% of coinfected cells would be observed in Cell-8 cells (Fig. (Fig.5).5). This simulation result is consistent with our actual observations at 72 hpi, when most of the infected sites show absolute spatial separation by 7 to 9 cell-to-cell movements (Fig. (Fig.2D),2D), indicating that our model and the estimated sizes of the bottlenecks are reliable.
As we observed, rapid spatial separation occurs between two artificial vector genomes during the development of locally infected regions by a plant virus. This phenomenon can be explained by the idea that rapid fixation of an allele occurs in bottlenecked populations (15). We extended this idea to model the rapid selection of trans-acting genes or elements in plant RNA viral genomes.
Some of the sources of genetic information in RNA viral genomes, such as 5′ and 3′ untranslated regions (UTRs), work in cis to the viral genomes, while others, such as MP and p19 of SBWMV expressed from subgenomic RNAs, work in trans. These trans-acting elements or gene products should be shared among intracellular populations of viral genomes. Thus, the selection of trans-acting genes or elements should be slow compared to the selection of cis-acting genes or elements because of complementation by adaptive genomes for defective ones in intracellular populations. We speculated that narrow genetic bottlenecks would solve this problem by stochastically isolating adaptive genomes from defective genomes, allowing adaptive genomes to benefit exclusively from the mutations in their genomes (Fig. (Fig.6A).6A). Therefore, we investigated how bottleneck sizes affect the speed of selection on trans-acting genes or elements by modeling the competition between intracellular populations, among which narrow bottlenecks create variety in the ratios of adaptive genomes to defective genomes.
Competition between intracellular populations was modeled by different probabilities of establishment of infection in adjacent cells: the probabilities of succession of intracellular populations (S). S was described by logistic curve with respect to the proportion of adaptive genomes in the intracellular population
Here Ne (effective population number) is the size of the bottleneck (i.e., the number of viral genomes that establish infection, MOI) and A is the number of adaptive genomes in total Ne genomes. We assumed a0 = 0.3 and c = 30; a0 and c determine the inflection point and inclination of the logistic curve, respectively. We used a0 = 0.3 because an SBWMV RNA2 mutant with ~30% transcription efficiency of p19 subgenomic RNA compared to that of wild-type virus could infect plants but showed irregular formed lesions (34), indicating that the virus can infect some cells but not others. With these parameter values, the succession probability of intracellular probability is very low if the frequency of the adaptive genome is below 0.2, while it is close to 1 if the frequency is over 0.4 (Fig. (Fig.6B6B).
The ratio of cells infected by A adaptive genome and Ne−A defective genomes in Cell-N was described as follows:
Assuming that there are abundant cells to receive intracellular populations, the ratio of adaptive genomes to the total population of Cell-N cells was described as follows:
Using the above model, exclusion of defective mutant genomes was tested. Starting from a mixed virus population with 80% adaptive genomes and 20% defective genomes (i.e., , rapid exclusion of the defective genome was observed for smaller Ne values (e.g., 5 or 10), while almost no change was observed for larger Ne values (e.g., 50 or 100) in 10 cell-to-cell movements (Fig. (Fig.6C).6C). Similarly, selection of an adaptive mutation was tested. Starting from a mixed virus population with 20% adaptive genomes and 80% defective genomes (i.e., = 0.2), rapid occupation by the adaptive genome was observed for smaller Ne values (e.g., 5 or 10), while a slower change was observed for larger Ne values (e.g., 50 or 100) (Fig. (Fig.6D).6D). On the other hand, a similar simulation modeling selection of cis-acting elements between adaptive genomes and less-adaptive genomes with 1:0.5 replication efficiencies showed that selection would rapidly occur almost independently of the size of bottlenecks (data not shown). We also confirmed that the simulation results are not largely affected by changing a0 and c (data not shown).
By observing the spatial separation of virus vectors carrying two different fluorescent proteins, we have shown that narrow genetic bottlenecks occur during cell-to-cell movement of a plant RNA virus in the leaves of the natural host and local lesion host. The estimated size of bottlenecks was surprisingly small, with averages of 5.97 ± 0.22 for first cell-to-cell movement and 5.02 ± 0.29 for second cell-to-cell movement. The underestimation effect of deletion mutations in fluorescent protein coding regions should be around 3 to 4% at the time points we carried out estimations (i.e., 22 and 28 hpi), because only fewer than 10% of deletion mutants were observed at 72 hpi. The estimated sizes of the bottlenecks are similar to those in the recent report by Gonzalez-Jara et al. (10), which showed that the MOI in plant tissue colonization (i.e., the size of bottlenecks) decreases from 6 to 1 to 2, corresponding to the expansion of the TMV-infected regions. The similarity of their and our estimated sizes indicates that narrow genetic bottlenecks in cell-to-cell movements are generally occurring with plant RNA viruses that infect mesophyll cells. However, we consider it difficult to say that decreases in the size of bottlenecks are generally occurring phenomena, because the estimations are affected by how we model the plant tissues. For example, we carried out our estimation assuming that the number of Cell-1 cells per an infected Cell-0 cell is eight and obtained λ1 = 5.97 ± 0.22 and λ2 = 5.02 ± 0.29; however, if we assumed the number is six or seven, we would obtain λ1 = 5.86 ± 0.29 and λ2 = 5.72 ± 0.38 or λ1 = 6.02 ± 0.25 and λ2 = 5.19 ± 0.30, respectively, indicating that there are negative relationships between the estimated sizes of the latter bottleneck and the assumed ratios of newly infected cells to source cells. Gonzalez-Jara et al. (10) carried out their estimations assuming that the ratio is always 6.5, but according to our understanding, as this ratio will rapidly decrease to almost 1 corresponding to the expansion of the infected regions (for two models to suggest the decrease in the ratio, see Fig. S2 in the supplemental material), they may have underestimated the sizes of bottlenecks at later time points. Accumulation of deletion mutations may also cause an underestimation of the sizes of bottlenecks at later time points. On the other hand, our model may slightly overestimate the sizes of bottlenecks because of the simplification that infection of a single cell occurs by founder genomes from an adjacent single infected cell. Thus, the changes in the sizes of bottlenecks during host colonization should be discussed further, especially with more attention paid to the way to model plant tissues, accumulation of deletion mutants, and spread of virus infection.
We do not know the mechanisms of the occurrence of the bottlenecks during cell-to-cell movement. However, we speculate that the bottleneck may not be a physical matter in cell-to-cell movement, because the number of plasmodesmata connecting two mesophyll cells is estimated to be 26, on average, using spinach leaves (31), which belong to the same family with C. quinoa, Chenopodiaceae, indicating that there are enough plasmodesmata for the virus to go through. Studies of replication complexes of hepatitis C virus (HCV) (32) and virus-induced mini-organelles, in which viral replication occur, of Flock House virus (FHV) (16) have shown that several hundred replication complexes and around 11 thousand virus-induced mini-organelles are formed when the viruses infect a host cell. Comparing the estimated bottleneck sizes with these results, it is reasonable to consider that the bottleneck event (i.e., the settlement of the founder virus) occurs prior to the formation of replication complexes or virus-induced mini-organelles. From this viewpoint, competition for resources required for genome replication or protein expression can be also excluded from the mechanisms of the bottleneck, because the bottleneck events seem to occur before the viral replication and protein expression become vigorous. As demonstrated by previous research on WSMV bottlenecks in systemic movement (11), bottlenecks during cell-to-cell movement may also occur due to sequence homology, probably via an RNA silencing mechanism to refuse additional infection by a virus with sequence homology. This idea can explain the fact that SBWMV does not suffer from narrow genetic bottlenecks in spite of its bipartite genome, because only a limited bottleneck effect between RNA1 and RNA2 will be expected. Further studies of the mechanisms and the timing of the occurrence of genetic bottlenecks are required.
Previous research on bacteriophage (4, 6) and animal (7, 8, 36) and plant (5) RNA viruses showed that repeated bottleneck events, caused by transferring plaques or lesions, resulted in fitness losses for viral genomes because of the mechanism known as Muller's ratchet (21). Our observations and estimations showed that intracellular populations of a plant virus face narrow genetic bottlenecks in every cell-to-cell movement, and, following this idea, bottlenecks should cause extinction or very low mean fitness of the populations. This may be the case for the history of an intracellular population traveling from one cell to another cell. However, because there are abundant cells and spaces for local infection in a host plant to receive viral intracellular populations, stochastically adaptive genomes persist or appear, and survival of the viral population as a whole will be achieved. Why have plant viruses not evolved to avoid bottlenecks? We speculate that the plant viruses are actually utilizing the bottlenecks as an essential element of their evolution mechanisms. In this study, we focused on viral elements working in trans to their genomes, which would not receive selection pressure as effectively as cis-acting elements because of the complementation in intracellular populations. Simulating this situation by describing competition among intracellular populations, our model implied that narrow genetic bottlenecks during cell-to-cell movement help the selection pressure to work on trans-acting genes or elements by rapidly isolating the adaptive genomes from defective genomes. This system may counteract the negative effect of bottlenecks (i.e., fitness losses), and, furthermore, it may enable the plant RNA virus to rapidly respond to changes such as temperature shift, condition changes in different organs of a host, host shifting and so on. Interestingly, a study of ϕ6, a lytic RNA bacteriophage, showed that repeated large population transfers with broadened bottlenecks result in occupation of the viral population by “selfish” genomes, each of which cannot effectively replicate by itself but can replicate well only among the intracellular population because of complementation (30). A similar situation could occur in plant RNA virus infection of a host plant if the bottleneck sizes in cell-to-cell movement were large, resulting in ineffective plant-to-plant transmission because of the bottlenecked transmission of selfish genomes, each of which cannot replicate well by itself. Thus, roughly constant but variable bottleneck sizes in cell infection through their life cycles (i.e., cell-to-cell movement, vascular to mesophyll cell invasion, and so on) may be favored for plant RNA virus evolution.
In conclusion, we demonstrated narrow genetic bottlenecks and their estimated sizes during cell-to-cell movement of a plant virus, and we created a simple model to explain why plant RNA viruses do not suffer from the bottlenecks. We believe this work provides a new insight into survival strategies and population dynamics of plant RNA viruses.
We thank Yukio Shirako (ANESC, Univ. of Tokyo) for providing us with infectious cDNA constructs for SBWMV, pJS1 and pJS2, used in this study. We also thank anonymous reviewers for critical and constructive comments, which improved the manuscript significantly.
S.M. was supported by the Japan Society for the Promotion of Sciences (JSPS) Research Fellowships for Young Scientists (20-5665) and the Japan Science Technology Agency (JST) PRESTO program. H.K. was supported by a Grant-in-Aid for Scientific Research (B-19300094) from JSPS.
Published ahead of print on 2 December 2009.
§Supplemental material for this article may be found at http://jvi.asm.org/.