Bacteria can become dormant or form spores when they are starved for nutrients. Here, we find that non-sporulating Bacillus subtilis cells can survive deep starvation conditions for many months. During this period, cells adopt an almost coccoid shape and become tolerant to antibiotics. Unexpectedly, these cells appear to be metabolically active and show a transcriptome profile very different from that of stationary phase cells. We show that these starved cells are not dormant but are growing and dividing, albeit with a doubling time close to 4 days. Very low nutrient levels, comparable to 10,000-fold diluted lysogeny broth (LB), are sufficient to sustain this growth. This extreme slow growth, which we propose to call ‘oligotrophic growth state’, provides an alternative strategy for B. subtilis to endure nutrient depletion and environmental stresses. Further work is warranted to test whether this state can be found in other bacterial species to survive deep starvation conditions.
Bacteria encounter multiple environmental stresses during their life, including depletion of nutrients. Some genera, such as Bacillus, Streptomycetes, and Clostridia, have developed specialized cells, spores, to survive extended periods of nutrient depletion. These dormant spores contain a dehydrated cytoplasm encased in a highly protective multilayer spore coat, making them resistant to extreme environmental conditions1. However, the majority of bacterial species do not form spores but are nevertheless able to survive prolonged periods of nutrient starvation. For example, the fish pathogen Flavobacterium columnare remains viable after 14 days of incubation in pure water2. Brucella suis, the causative agent of swine brucellosis, can survive 6 weeks of incubation in a salt solution3, and Escherichia coli can withstand 260 days of incubation in river water4. It should be mentioned that in all these cases it was only a small fraction of the population that survived. Cells that are exposed to deep starvation conditions typically show morphological changes, e.g. coiling in the case of F. columnare cells2, and cell shrinkage in the case of Micrococcus luteus and Staphylococcus aureus5,6.
A recurring question is how dormant these long-term starved cells are. In contrast to bacterial spores, which are fully dormant, it is likely that starved non-sporulating cells have to maintain some basic cellular activities, such as the proton motive force, to remain viable. For example, S. aureus cells starved for 7 days showed some sensitivity toward chloramphenicol indicating ongoing translation6. On the other hand, Mycobacterium tuberculosis starved for 6 weeks tolerated extensive treatment with the RNA polymerase inhibitor rifampicin or the mycobacterial cell wall synthesis inhibitor isoniazid, suggesting a fully dormant state7.
The soil bacterium Bacillus subtilis forms dormant endospores upon prolonged nutrient starvation. Sporulation is a costly differentiation process in terms of time and energy, and cannot be reversed once the asymmetric sporulation septum has been formed8,9. That is why B. subtilis only initiates sporulation in a fraction of cells in a population10. This differentiation bifurcation is known as a bet-hedging strategy, as it enables the population to survive when starvation continues or to quickly respond when there is an influx of fresh nutrients11,12. However, this bifurcation raises the question what happens with the non-sporulating cells when the starvation period continues.
In this study we show that non-sporulating B. subtilis cells can survive for many months in pure water, and that they become tolerant to different stresses. Using cell biological techniques and a novel assay for growth, we were able to demonstrate that these cells are not dormant but instead are growing slowly. Transcriptome profiles of these cells differed substantially from exponentially growing and stationary phase cells, indicating that these cells undergo an alternative cellular adaptation process. We propose to call this the “oligotrophic growth state”. The advantage of this cellular differentiation over sporulation and whether oligotrophic growth is a common mechanism in bacteria to survive prolonged nutrient depletion are further discussed.
Survival of non-sporulating B. subtilis
To facilitate the examination of non-sporulating B. subtilis cells, we made use of a sporulation-deficient mutant. Sporulation begins with phosphorylation of the response regulator Spo0A13. Since this transcription factor regulates many other stationary phase processes, including biofilm formation, genetic competence, and degradative enzyme production14, we left the spo0A gene intact and instead used a strain with an impaired spoIIE gene, which is one of the first essential sporulation genes induced by Spo0A, and is not required for other differentiation processes15. The ∆spoIIE strain was grown in Spizizen minimal medium (SMM) at 37 °C under continuous shaking. Samples were withdrawn at regular time intervals to determine viability by measuring colony-forming units (CFU). Unexpectedly, this non-sporulating strain not only survived several days without fresh nutrients, but even after 100 days the culture still contained some viable cells that formed colonies (Fig. 1a).
In the stationary growth phase unused amino acids are left in the medium and substantial levels of overflow metabolites accumulate. Moreover, we observed a drop in optical density and in CFUs during the first 2 days of starvation (Fig. 1a), suggesting a release of more nutrients. To be sure that these nutrients could not be used for further growth, cultures were filtered after 2 days of stationary growth and subsequently resuspended in a modified SMM lacking any carbon source, here called starvation buffer. This deep starvation procedure, schematically outlined in Supplementary Figure 1, was used in all further experiments. In this starvation buffer, deprived of any nutrients, non-sporulating B. subtilis cells still survived for more than 100 days (Fig. 1b). The pH remained stable for at least the first 14 days, which is not surprising considering the presence of 100 mM phosphate buffer. However, even when cells were resuspended in pure water they also survived, although with lower CFU counts (Fig. 1b). Clearly, B. subtilis cells can survive prolonged nutrient starvation conditions without having to resort to sporulation.
To confirm that non-sporulating B. subtilis cells are also present in wild-type populations under deep starvation conditions, the number of sporulating and non-sporulating cells was monitored in a wild-type B. subtilis culture. As shown in Fig. 1c, eventually most cells sporulated, however, a substantial fraction of the population (~20–30%) comprised non-sporulating cells, even after more than 100 days of deep starvation. For the first 14 days of starvation, this was confirmed by counting spores and non-sporulating cells by phase contrast microscopy (Supplementary Figure 2B). Comparable results were found when a wild-type culture was resuspended into pure water (Supplementary Figure 2C).
B. subtilis spores can germinate spontaneously even when conditions are unfavorable for growth. It is assumed that by this mechanism spores can scout the environment16. To examine whether there is a germination-sporulation cycle during long starvation conditions, we measured the viable count of a mutant that is unable to germinate17. During the first 11 days of starvation, this strain followed the same reduction in viable counts as the non-sporulating ∆spoIIE strain. After that the viable count reduced approximately one more log-unit and stabilized around 104 CFU ml−1 (Supplementary Figure 3). The extra reduction in viable counts after 11 days suggests that a fraction of the germination mutant formed spores. However, this reduction did not continue, at least for another 40 days (Supplementary Figure 3), indicating that B. subtilis does not use a continuous sporulation-germination cycle to survive long-term starvation. Thus, in contrast to the general assumption, B. subtilis does not necessarily have to sporulate to survive long periods of nutrient starvation. For reasons of practicality, the rest of the starvation experiments were performed with the non-sporulating ∆spoIIE strain, and CFU measurements were limited to 14 days’ incubation in starvation buffer.
Morphological changes caused by long-term nutrient deprivation, primarily a reduction in cell size, have been observed for several bacterial species2,5,6. When a B. subtilis ∆spoIIE culture was filtered and incubated in starvation buffer, we noticed a 40% reduction in cell length over the first 2 days, and cells became almost coccoid (Fig. 2a, b). It should be mentioned that the time axis in Fig. 2b depicts the days of incubation in starvation buffer after filtration. Consequently, at time point day 0 cells have already undergone 2 days of stationary phase in the SMM.
The reduction in cell length in the first 2 days of deep starvation suggested that the starved cells are still able to divide. After the cells became so short that they reached an almost coccoid shape, the cell length remained constant (Fig. 2b). This raised the question how metabolically active these small non-sporulating cells are when they have been incubated for up to 2 weeks in buffer lacking any nutrients. Previous studies used antibiotic sensitivity as an indication of metabolic activity in starved cells6,18. The addition of chloramphenicol to starved non-sporulating B. subtilis cells had no effect on survival (Fig. 3a). Ampicillin efficiently killed exponentially growing cells, but nutrient-starved cells were much more tolerant to this bactericidal antibiotic (Fig. 3b). A starvation period of 7 and 14 days also resulted in an increased tolerance to paraquat, an inducer of oxidative stress19 (Fig. 3c).
These data suggested that the small coccoid-shaped B. subtilis cells are dormant. To test whether these cells still maintain a membrane potential, cells were treated with the membrane potential-dissipating ionophore valinomycin. This led to a clear decrease in CFUs (Fig. 3d). When we measured the membrane potential in individual cells using the voltage-sensitive dye 3,3′-dipropylthiadicarbocyanine iodide (DiSC3(5))20, deep-starved cells appeared to have a membrane potential levels almost comparable to those found in exponentially growing cells (Fig. 3e).
Protein synthesis capacity
The presence of a membrane potential strongly suggests that the deep-starved cells are still metabolically active. To test whether these cells are capable of expressing proteins, an isopropyl β-d-1-thiogalactopyranoside (IPTG)-inducible green fluorescent protein (GFP) reporter fusion was introduced into the cells. Samples of 0-, 7-, and 14-day-starved cultures were taken and incubated with 1 mM IPTG for 4 h after which GFP levels were measured using fluorescence light microscopy. Surprisingly, 14-day-starved cells were expressing GFP, and in fact better than day 0 cells (Fig. 4). Apparently, the protein synthetic machinery is better adapted to starvation conditions after several days than at the onset of starvation.
To confirm that starved cells were metabolically active, we determined nascent peptide synthesis in individual cells by incubation with the amino-acid analog l-homopropargylglycine (L-HPG) for 18 h followed by fluorescent labeling with Alexa594 using click chemistry21. Alexa594 levels in individual cells was measured using fluorescence light microscopy and showed a clear accumulation of the fluorophore in 14- and 19-day-starved cells further incubated with L-HPG (Supplementary Figure 6A, B). Heat-inactivation (15 min 80 °C) or the addition of 200 μg ml−1 puromycin completely blocked the incorporation of L-HPG. Finally, we labeled nascent peptidoglycan using the fluorescent d-amino acids analog NBD-amino-d-alanine (NADA)22, and found that the cell wall of starved cells showed a clear fluorescence after 24 h incubation with NADA (Supplementary Figure 6C). Together, these data show that the surviving cells are still metabolically active despite 2 weeks of starvation.
The small coccoid B. subtilis cells and classic stationary phase B. subtilis cells have in common that they show tolerance to antibiotics (e.g. Fig. 3, day 14 and day 0, respectively). This is not surprising since both types of cells are dealing with nutrient-limiting conditions that suppress growth. On the other hand, the small coccoid B. subtilis cells are capable of synthesizing high levels of protein (Fig. 4). To examine whether deep-starved B. subtilis cells differ from stationary phase cells, we performed an RNA-sequencing experiment to compare the transcriptome profiles of both cell types. To obtain sufficient cells after 14 days, a 1 l culture was used as starting material. For the comparison with stationary growth phase cells, a culture was grown in SMM and incubated overnight. The transcriptome profile of an exponentially growing culture was also included in the analysis. As shown in Fig. 5a, a principal component analysis indicated that the 14-day-starved cells differ substantially from both stationary phase and exponentially growing cells. This is also illustrated by a heat map of the transcriptome profiles (Fig. 5b). One hundred-sixty-five genes were at least twofold upregulated in the 14-day-starved culture when compared to the exponentially culture, and 145 genes were at least twofold upregulated in the 14-day-starved cultures when compared to the stationary phase cultures (Fig. 5c). Thirty of these genes were only upregulated in the 14-day-old cells (Table 1). The majority of these genes are involved in nutrient acquisition (araE, exuT, rbsC, rbsD, and rhiF) and utilization (acoABC, araBDLNPQ, ganB, hutH, manA, uxaC, and uxuA). Twenty-one genes were uniquely downregulated in the 14-day-old cells compared to both the exponential and stationary phase cells (Fig. 5c). The majority of these genes are involved in biofilm formation (bioI, epsD, epsI, epsJ, epsL, and tasA) or competence development (comC, comGC, comGD, comGE, comGF, and comGG) (Table 1).
Growth and cell division
The transcriptome data indicated that the 14-day-starved cells differed substantially from stationary phase cells, and the DiSC3(5) assay (membrane potential) and GFP induction experiments suggested that 14-day-starved cells are metabolically active. Also cell division genes, such as ftsZ, ftsA, ftsL, pbpB, and divIVA, were not downregulated in the 14-day-old culture compared to the exponentially growing culture. This forced us to consider the possibility that these 14-day-starved coccoid B. subtilis cells are not dormant but are actually growing. As a first test we examined the localization of the cell division protein DivIVA in deep-starved cells using a DivIVA-GFP reporter fusion. DivIVA is involved in cell division regulation and accumulates at midcell when synthesis of the division septum creates a strong concave (inward) curvature of the cell membrane to which DivIVA specifically binds23,24. Microscopic images of cells that had undergone 14 days of deep starvation showed a clear fluorescence signal at midcell, suggesting that these cells were still actively dividing (Fig. 6a). When we counted these cells, the frequency of midcell localized DivIVA-GFP seemed to increase during the first 7 days of deep starvation (Fig. 6b).
The presence of cell division proteins at midcell is no definitive proof for growth. To unequivocally determine whether long-term starvation resulted in dormant or in growing cells, we developed a new assay based on blocking cell division. The compound 3-methoxybenzamide (3-MBA) impairs polymerization of the key cell division protein FtsZ of B. subtilis, resulting in inhibition of cell division and consequently cell elongation25. In theory, this should reveal whether starved cells are either dormant or still growing. Samples were taken over a 14-day starvation period at regular time intervals and cells were incubated in the presence or absence of 3-MBA for 48 h. Cells were stained with the fluorescent membrane dye FM5-95 to facilitate cell length measurements (Fig. 7a). Consistent with the previous cell length measurements (Fig. 2), a reduction in cell length was observed for untreated day 0 samples after 48 h. As expected, this reduction was suppressed when cell division was blocked by 3-MBA. Interestingly, after 2 days of starvation the presence of 3-MBA resulted in a clear increase in cell length, and this was even the case for cells that were starved for 14 days (Fig. 7a, b). We also tested starved wild-type cells and found a similar result (Supplementary Figure 7A). 4′,6-diamidino-2-phenylindole staining of 3-MBA-treated cells showed that these elongated cells contained normal nucleoids (Supplementary Figure 7B), indicating that cell elongation is accompanied by chromosome replication. Importantly, when we tested an ftsZ mutant (G196S, N263K) that is resistant to 3-MBA26, no increase in cell length was observed (Supplementary Figure 7C). We must therefore conclude that deep starvation does not lead to dormant cells but to actively growing cells.
With an average increase in cell length of 0.75 µm after 48 h incubation with 3-MBA (Fig. 7b), and an average cell length of ~1.5 µm (Fig. 2), the doubling time of these deep-starved B. subtilis cells is estimated to be approximately 4 days. Since these cells show such a distinct transcriptome profile and cell shape, and since they are still growing, we propose to call this the “oligotrophic growth state”.
Oligotrophic growth implies the presence of small levels of nutrients in the starvation buffer. A likely source is the cells that lyse in the first days of incubation. To confirm this, 7-day-old cells were filtered and resuspended either in the filtrate or in fresh starvation buffer. As shown in Fig. 8a, resuspension in starvation buffer resulted in a further decline in the CFU, whereas resuspension in the culture filtrate had no effect on the CFU count. Clearly, cell lysis is necessary to provide nutrients to maintain the oligotrophic growth state of the surviving cells. This also explains why stationary phase cells, when filtered and resuspended into fresh starvation buffer (day 0 samples), displayed a lower membrane potential and a low capacity to express GFP than later time samples (Figs. 3e and 4).
A Bradford assay to quantify protein concentrations indicated that the amount of proteins released from lysed cells reached approximately 120 µg ml−1 after 4 days of starvation (Supplementary Figure 8). To confirm that this low concentration of proteins is indeed sufficient to support oligotrophic growth, 7-day-starved cultures were filtered and resuspended in starvation buffer containing low concentrations of either tryptone or peptone. It appeared that even concentrations as low as 0.5 µg ml−1 tryptone or peptone were sufficient to maintain the oligotrophic growth state (Fig. 8b).
To determine whether the oligotrophic growth state requires specific gene products, several of the upregulated genes in Table 1 were deleted (acoA, manA, mmgB, yezD, and yisJ) and tested for survival under deep starvation conditions. However, none of the five tested deletions reduced the viability (Supplementary Figure 9A).
Several of the upregulated genes in Table 1 are controlled by alternative sigma factors27,28. We first tested whether one of the sporulation sigma factors (∆sigE, -F, -G, -H, and -K) was required for survival, but none of the sigma factor deletion mutants showed an effect (Supplementary Figure 9B). Also mutants lacking either the general stress response sigma factor SigB, the heat shock sigma factors SigI, or the sigma factor SigL, which renders cells cold-sensitive, were able to survive for 14 days without problems (Supplementary Figure 9C). Last, we tested the extra-cytoplasmic function (ECF) sigma factors (SigM, -V, -W, and -X) involved in cell envelope stress29. As shown in Fig. 8c, the ∆sigX mutant showed a continuous decline in viable count, reaching an order of magnitude lower CFU counts after 14 days, suggesting that the oligotrophic cells are exposed to cell wall disturbing factors. To examine whether bacteriophages are responsible for this, we tested a strain lacking all six prophages30. However, this strain showed a reduction in CFUs that was comparable to the wild type (Supplementary Figure 9D). A strain lacking the major autolysin LytC, involved in cell separation and cell wall turnover, also had no strong effect on survival (Supplementary Figure 9D). We then examined whether the main stress proteins are necessary for survival and tested strains lacking either the protein quality control protease ClpP, the stringent response regulator RelA, or the DNA recombination/repair proteins RecA and PnpA31,32. Only the ΔrelA mutant showed a slightly lower viability after 7 and 14 days of deep starvation (Supplementary Figure 9D).
Differentiation processes in B. subtilis are coordinated by a few key transcription factors. Motility is activated by the sigma factor SigD, genetic competence by the activator ComK, and transcription factors like SinI, CodY, AbrB, DegS, DegU, and Spo0A regulate differentiation processes such as sporulation, degradative enzyme production, and biofilm formation10,33,34. However, none of these transcription factors were essential to survive deep starvation, although the absence of DegU caused a reduction in viable count, especially during the first week of starvation (Fig. 8d). The response regulator DegU controls expression of secreted proteases and it is likely that proteases are necessary for the release of nutrients from lysed cells. Indeed, a strain lacking all eight extracellular secreted proteases (strain ∆WB800 lacking nprB, aprE, epr, bpr, nprE, mpr, vpr, and wprA)35 showed a 100-fold decrease in survival (Fig. 8e). To determine whether this was due to the absence of a specific protease, we introduced sequential deletions of the eight protease genes into the spoIIE background. As shown in Fig. 8f, only the strain lacking all eight proteases showed a decrease in viable count. wprA was the last deleted gene (∆8) but a single wprA deletion (∆wprA) showed normal CFU levels (Fig. 8f). This demonstrated that a single secreted protease is sufficient for oligotrophic growth. We also tested whether the absence of the extracellular nucleases NucA or NucB made a difference, but this was not the case (Fig. 8e).
Salt resistance and escape
Oligotrophic environments are ubiquitous and include most lakes and seas, but can also be found in soil36. In fact, B. subtilis is not only found in soil but can also be isolated from seawater37. When we used artificial seawater for deep starvation experiments, the viability increased, and CFU counts became 10× higher, indicating that B. subtilis can maintain oligotrophic growth in salty seawater (Fig. 8g).
Finally, we tested how much time it takes for cells to escape the oligotrophic growth state and resume normal growth. To this end, samples from 14-day-starved cultures were inoculated in fresh SMM medium. For comparison, normal stationary phase cells were used that were grown overnight in SMM medium. The overnight culture was diluted 103 times to obtain comparable viable counts at t = 0. Growth was followed by either viable count measurements or optical density in microtiter plates. As shown in Fig. 8h, the 14-day-starved cells resumed growth as efficiently as cells from the overnight culture. Thus, cells in the oligotrophic growth state are capable of rapidly responding to improved nutrients conditions.
A recurring question is whether cells become dormant when exposed to long-term starvation conditions or whether they are still metabolically active. The main reason for this is that an unambiguous assay for (very slow) cell growth has been lacking. One of the longest microscopic observations, 1.5 days monitoring of starved E. coli cells in a microfluidic setup, did not detect cell growth38. On the other hand, in a long (weeks) starvation experiment using E. coli, mutants appeared that could outcompete non-starved cells, suggesting that starved cells were still active39. However, it should be noted that in this experiment the starved cells were kept in the same growth medium (lysogeny broth (LB) medium) and were not resuspended in fresh water or buffer lacking any nutrients. Other long-term starvation studies, e.g. with M. luteus, Deinococcus sp., and E. coli, concluded that deep starvation resulted in dormant cells5,40,41. Prolonged nutrient starvation can also result in viable-but-non-culturable (VBNC) cells42,43,44. These VBNC cells appear metabolically active when observed with certain fluorescent probes, but they can no longer grow when nutrients are replenished45. In our experiments the drop in CFU appears to be caused primarily by cell lysis rather than the appearance of VBNC cells, since the optical density of starved cultures decreased substantially and microscopic observations also showed a strong reduction in cell numbers.
Here we have shown that deep starvation of B. subtilis results in actively growing cells, however this growth does not lead to an increase in CFUs. This balance between cell growth and cell lysis has been coined cryptic growth46. This phenomenon is presumably widespread in nutrient-depleted cultures but it is difficult to measure, and previously could only be assessed indirectly by testing sensitivity toward antibiotics or the incorporation of radioactive precursors. Our cell division inhibition assay with 3-MBA provides now an unambiguous test for cryptic growth, enabling direct detection of slow growing cells at a population-wide scale.
A fascinating question is how cell growth and cell lysis are balanced during cryptic growth. In B. subtilis, the matured endospore escapes the mother cell by programmed cell lysis47. In addition, B. subtilis cells can display a cannibalism phenotype during stationary phase, releasing killing factors that specifically lyse other B. subtilis cells, thereby releasing nutrients into the medium48. Whether these mechanisms are involved in cryptic growth-related cell lysis remains to be determined. However, both cell lysing mechanisms are activated by Spo0A, and since a ∆spo0A mutant shows the same lysis pattern as wild-type cells, other mechanisms might be active. We can rule out the involvement of bacteriophages, given that a strain devoid of all bacteriophages showed a normal oligotrophic growth pattern (Supplementary Figure 9D). It has been shown that depletion of the proton motive force causes autolysis of B. subtilis cells49. After 14 days of deep starvation, the membrane potential is almost comparable to that of normally growing cells in many cells. However, there is a large heterogeneity in membrane potential levels (Fig. 3e), and it is possible that cells with low membrane potentials are the ones that are prone to lysis.
The oligotrophic B. subtilis cells showed an increased tolerance to chloramphenicol, ampicillin, and oxidative stress. Tolerance to environmental stresses during nutrient deprivation is well-known. For example, starved E. coli and Vibrio cells have been shown to become tolerant to hydrogen peroxide, heat, and ultraviolet (UV) radiation50,51. Starved S. typhimurium cells develop tolerance to UV radiation and hydrogen peroxide, as well as tolerance to acids52. Tolerance to antibiotics by reduction of the growth rate has been put forward as the main reason for the bacterial persister phenotype53. During oligotrophic growth of B. subtilis the doubling time is reduced more than 100× compared to normal exponentially growing cells (from ~40 min to ~4 days). This dramatic reduction in growth rate might explain why oligotrophic cells are tolerant to chloramphenicol and ampicillin and cope better with oxidative stress. This property might also explain why mutants with either reduced DNA repair (∆recA), cold shock survival (∆pnpA), protein refolding (∆clpP), or general stress survival (∆sigB) capacities did not show a decrease in viability during the 14 days’ starvation.
Whether oligotrophic growth is a carefully regulated differentiation process remains to be seen. Of the transcriptional regulators tested in this study, only the absence of SigX, DegU, and RelA showed an effect on viable counts during starvation. However, the absence of the stringent response regulator RelA, and the two-component response regulator DegU involved in the induction of secreted proteases, had only mild effects on survival. The strongest effect, one order of magnitude reduction in viable count after 14 days, was observed for the ΔsigX mutant. The ECF sigma factor SigX induces genes that modify the cell wall, making cells more resistant to heat and certain cell envelope-targeting compounds54,55.
Oligotrophic cells have to be thrifty and the turnover of proteins will be slow, as the tolerance against chloramphenicol indicated. In addition, the extreme reduction in growth rate means that for most processes only a limited number of proteins are required to fulfill the necessary tasks. This is for example illustrated by the fact that only a single protease is required to maintain oligotrophic growth (Fig. 8f). Transcription is an intrinsically noisy process56 and some leaky expression will occur especially over long time intervals. Therefore, a carefully regulated signal transduction pathway might not be essential in these slowly growing cells, and substrate feedback at the enzyme level might be the predominant measure of regulation during oligotrophic growth.
Some bacteria are obligate oligotrophs whereas others are facultative oligotrophs57. B. subtilis can now be added to the latter family. We have shown that concentrations as low as 0.5 µg ml−1 tryptone or peptone are sufficient to maintain oligotrophic growth. Normally, B. subtilis is studied using rich growth media such as LB. LB is composed of 10 mg ml−1 tryptone and 5 mg ml−1 yeast extract, thus, concentrations that are approximately 10,000 times higher than necessary for oligotrophic growth. Since B. subtilis lives in oligotrophic environments such as soil and seawater, the question arises whether growth in rich media like LB is the most natural condition to investigate this organism, and whether oligotrophic growth might not be the most common cellular state of this organism in nature.
It will be interesting to see whether oligotrophic growth is a common survival strategy for bacteria. A large drop in CFU during the first days of deep starvation is observed for most bacteria that are starved for prolonged periods of time, including S. aureus, E. coli, M. luteus, S. typhimurium, B. suis, and F. columnare2,3,6,58,59. Consequently, at least the small amount of nutrients necessary to support oligotrophic growth will be available.
Thus far, sporulation has been considered the principal cellular differentiation through which B. subtilis survives prolonged periods of nutrient depletion. Here we show that B. subtilis can also survive by growing very slowly, a state that makes them resilient to a variety of environmental stresses. The advantage of oligotrophic growth over sporulation is that oligotrophic cells are able to rapidly resume normal growth when nutrient conditions improve (Fig. 8h), whereas spore germination is a time-consuming and extremely heterogenic process, with many spores delaying outgrowth even when conditions are good16,60. In conclusion, oligotrophic growth adds another differentiation state to the already rich repertoire of cellular differentiations that B. subtilis is capable of.
Maintenance and growth of strains
Nutrient agar (NA) (Oxoid) was used for routine selection and maintenance of both B. subtilis and E. coli strains. Supplements were added as required: chloramphenicol (cm, 5 and 50 µg ml−1), erythromycin (erm, 1 µg ml−1), kanamycin (kan, 2 μg ml−1), spectinomycin (spec, 50 µg ml−1), tetracycline (tet, 10 µg ml−1), ampicillin (amp, 100 and 1000 µg ml−1), valinomycin (val, 10 and 100 µM), IPTG (1 mM), and paraquat (para, 100 and 1000 µM). For liquid cultures, cells were cultured in either SMM61 (15 mM (NH4)2SO4, 80 mM K2HPO4, 44 mM KH2PO4, 3 mM tri-sodium citrate, 0.5% glucose, 6 mM MgSO4, 0.2 mg ml−1 tryptophan, 0.02% casamino acids, and 0.00011% ferric ammonium citrate (NH4)5Fe(C6H4O7)2), LB (10 g l−1 tryptone, 5 g l−1 peptone, and 10 g l−1 NaCl), or Penassay broth.
Strains and primers used in this study are listed in Supplementary Table 1 and 2, respectively. Strain construction was achieved through transformation of recipient strain with chromosomal DNA from the appropriate strain, and checked by selecting for the correct resistance. For strain DG034, the erythromycin resistance cassette was removed using plasmid pDR244 according to the protocol provided by the Bacillus Genetic Stock Center. Briefly, pDR244 was transformed into the recipient strain and selected for at 30 °C on spectinomycin. Successful colonies were then streaked onto plain NA plates and incubated at 42 °C overnight. The resultant colonies were then checked for sensitivity to both spectinomycin and erythromycin. The removal of the cassette was confirmed by PCR. All strains containing “clean” gene deletions, no antibiotic resistance marker, were verified by PCR using oligonucleotides listed in Supplementary Table 2. In order to replace the erythromycin resistance cassette in strain PG344, marker-exchange using plasmid pErm::Spec was carried out62.
Deep starvation conditions and spore assay
Bacteria were cultured in SMM at 37 °C with aeration for 48 h. Cells were collected by vacuum filtration using a 47-mm filter membrane with 0.45-µm pores (Thermo Fisher Scientific). This was always performed at 37 °C to prevent temperature shock. Filtered cells were resuspended in starvation buffer (15 mM (NH4)2SO4, 80 mM K2HPO4, 44 mM KH2PO4, 50 mM NaCl, and 0.8 mM MgSO4) by vortexing. The resuspended cultures were incubated at 37 °C while shaking for 14 days. Periodic sampling was performed to determine viable counts through serial dilutions and plating on NA plates. The spoIIE gene was deleted by insertion of an erythromycin resistance marker. This, and the use of the DivIVA-GFP marker in several cases, enabled us to check for possible contaminations during long starvation periods.
Spore numbers were determined by heating samples for 25 min at 80 °C, which will kill normal cells except for spores. A serial dilution on NA plates was used to determine spore counts.
Microscopic experiments were performed using a Nikon Eclipse Ti (Nikon Plan Fluor ×100/1.30 Oil Ph3 DLL and Plan Apo ×100/1.40 Oil Ph3 objectives) microscope. Images were acquired using Metamorph 6 (Molecular Devices, Inc) and analyzed with ImageJ (National Institutes of Health). For visualization, 0.3 µl samples were immobilized on a thin layer of 1.2% agarose and a glass coverslip (VWR) was placed on top.
Cell lengths were determined by staining cell membranes with 0.4 µg ml−1 FM5-95 (Molecular Probes), followed by length measurements using ImageJ. To determine changes in cell length, samples were treated with 10 µM of the FtsZ inhibitor 3-MBA for 48 h at 37 °C. Images were acquired at the beginning of incubation and after 48 h.
GFP levels were determined using a GFP-filter set and quantification using ImageJ. On days 0, 7, and 14 of starvation strain DG017 (amyE::spec Phyperspank-sfGFP) was incubated with and without 1 mM IPTG for 4 h at 37 °C, after which cells were observed with fluorescence light microscopy.
Membrane potential determination was achieved using the voltage-sensitive dye DiSC3(5), which accumulates in polarized cells20. Cellular membrane potential levels were assessed for starved cells by incubating cells with 2 µM DiSC3(5) for 5 min at 37 °C, followed by microscopy using Cy5-filter sets. As a control, the DiSC3(5)-fluorescence levels were measured for exponentially growing cells, and cells depolarized with 10 µg ml−1 gramicidin ABC20.
To determine nascent peptide synthesis, samples were treated with 1 mM of the amino-acid analog L-HPG (Jena Bioscience) for 18 h at 37 °C. The samples were washed with 1× phosphate-buffered saline and subsequently permeabilized using sequential resuspension in 50 and 100% ethanol. The L-HPG incorporated in the nascent peptides was clicked to the azide group in AF594-azide (Jena Bioscience) using click chemistry21, using THPTA-based CuAAC Cell Reaction Buffer Kit (Jena Bioscience). Cells from microscopy images were auto-selected and quantified using Coli-Inspector63. Statistical analysis between HPG+ and other control samples was performed using unpaired t-test in GraphPad Prism.
To visualize peptidoglycan synthesis, fluorescently labeled d‐amino acid NADA was used22. Efficient peptidoglycan labeling of B. subtilis cells requires a strain lacking the d,d‐carboxypeptidase encoded by dacA22. ∆dacA (strain DacAKS15) cultures were set up in accordance with the starvation protocol. After 7 and 14 days of starvation, 400 µl samples were taken and incubated with and without 5 µM NADA for 48 h at 37 °C. From these subcultures 100 µl samples were taken after 1 and >24 h. The cells underwent a centrifugation wash, to remove excess NADA, and resuspended in starvation buffer, after which cells were observed with fluorescence light microscopy.
B. subtilis (ΔspoIIE) cultures were set up in accordance with the starvation assay. In order to obtain sufficient cell material, 1 l culture volumes were used. Cells were collected by filtering through 90-mm polyethersulfone membrane filters (0.22-µm pores (Millipore)) at 37 °C. For comparison, stationary phase and exponential phase cells were collected. For stationary growth phase samples, 1 l ΔspoIIE cultures were grown overnight (16–18 h) at 37 °C under continuous shaking. For the exponential growth phase samples, 1 l ΔspoIIE cultures were grown to an OD600 of ~0.2 at 37 °C under continuous shaking. Also the stationary phase and exponential growing cells were collected by filtration. After harvesting cells were flash-frozen in liquid nitrogen, and stored at −80 °C.
To isolate RNA, the frozen pellets were grounded by using a mortar and pestle before immersion in QIAzol Lysis Reagent (Qiagen). RNA was isolated and purified using the RNeasy kit (Qiagen), including an on-column treatment with the RNase-free DNase set (Qiagen). The concentration was measured on a NanoDrop ND-2000 (Thermo Scientific) and RNA integrity was examined using the 2200 TapeStation System with Agilent RNA ScreenTapes (Agilent Technologies). ERCCs spike-in mix 1 (Thermo Fisher Scientific) were added to each RNA sample and a ribosomal RNA depletion was performed using the Ribo-Zero rRNA Removal Kit (Gram-Positive Bacteria) (Illumnia). Barcoded RNA libraries were generated according to the manufacturers’ protocols using the Ion Total RNA-Seq Kit v2 and the Ion Xpress RNA-Seq barcoding kit (Thermo Fisher Scientific). The size distribution and yield of the barcoded libraries were assessed using the 2200 TapeStation System with Agilent D1000 ScreenTapes (Agilent Technologies). Sequencing was performed on the Ion Proton system using the Ion PI Chips (Thermo Fisher Scientific) according to the manufacturers’ protocols.
The quality of the sequencing data was assessed using FASTQC64 and an in-house pipeline. The reference genome and annotation were downloaded from the NCBI (NC_000964.3), and the sequence reads were mapped onto the genome65. The gene expression levels were quantified using HTseq. The data were normalized and analyzed for differential expression using DESeq266. Gene expression data have been deposited at the public repository Gene Expression Omnibus, accession number GSE102140. Variance stabilized normalized data were subjected to principal component analysis and cluster analysis, using R statistical software.
Protein concentration of the starvation medium was determined using a Bradford assay (Bio-Rad) according to the manufacturers’ instructions. Samples from starvation cultures were taken through the incubation period, cells were removed by centrifugation (5 min at 8000 rpm, ~14,000 × g) and the supernatant used for the Bradford assay.
Both stationary phase cells and 14-day-old cells (∆spoIIE) were used to inoculate SMM (1:10 diluted). Stationary phase cells were first diluted 1000-fold in order to have approximately the same starting cell count as 14-day-starved cells. Cultures were incubated at 37 °C with aeration. The CFU was determined by taking periodic samples and serial dilution on NA plates. The OD600 was determined using a microtitre plate reader (BMG FLUOstar OPTIMA).
Further information on experimental design is available in the Nature Research Reporting Summary linked to this article.
Gene expression data have been deposited in the public repository Gene Expression Omnibus, accession number GSE102140. Other data supporting the findings of this study are included in the paper and its Supplementary Information files, or available from the corresponding author upon request.
Journal peer review information: Nature Communications thanks the anonymous reviewers for their contribution to the peer review of this work. Peer reviewer reports are available.
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We would like to thank S. Syvertsson, J. Kirstein, J. Stülke, R. Daniel, A. Guyet, J. Errington, T. Ewen, S. Ishikawa, and C. Harwood for strains; and K. Turgay for critical reading of the manuscript. Funding for D.A.G. was provided by a Biotechnology and Biological Sciences Research Council (BBSRC) DTP Studentship BB/J014516/1. G.D. was funded by EMBO (ALTF 936–2016) and European Commission MCSA-IF grant 749510. P.G. and H.S. were funded by BBSRC grants BB/I004238/1 and BB/I01327X/1, respectively, and L.W.H. was partially funded by STW-Vici grant 12128 from the Netherlands Organization for Scientific Research (NWO).