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CcrZ is a pneumococcal spatiotemporal cell cycle regulator that interacts with FtsZ and controls DNA replication by modulating the activity of DnaA

Abstract

Most bacteria replicate and segregate their DNA concomitantly while growing, before cell division takes place. How bacteria synchronize these different cell cycle events to ensure faithful chromosome inheritance by daughter cells is poorly understood. Here, we identify Cell Cycle Regulator protein interacting with FtsZ (CcrZ) as a conserved and essential protein in pneumococci and related Firmicutes such as Bacillus subtilis and Staphylococcus aureus. CcrZ couples cell division with DNA replication by controlling the activity of the master initiator of DNA replication, DnaA. The absence of CcrZ causes mis-timed and reduced initiation of DNA replication, which subsequently results in aberrant cell division. We show that CcrZ from Streptococcus pneumoniae interacts directly with the cytoskeleton protein FtsZ, which places CcrZ in the middle of the newborn cell where the DnaA-bound origin is positioned. This work uncovers a mechanism for control of the bacterial cell cycle in which CcrZ controls DnaA activity to ensure that the chromosome is replicated at the right time during the cell cycle.

Main

In many bacterial species, DNA replication and cell division occur concomitantly1,2,3. Different models exist to explain how Escherichia coli or Bacillus subtilis handle DNA replication together with cell division4,5,6,7. A current cell-size control model suggests that cells initiate DNA replication independently of their original size, and grow to a constant size independent of their size at birth (adder model)8,9,10,11,12. How cells sense changes in cell size and use this to trigger replication initiation is not known, but the models imply the existence of regulatory controls3,13,14,15. However, no such cell cycle regulator has been reported to date for bacteria.

Although E. coli and B. subtilis use different systems for regulating their cell cycles, the way they localize their division site is conserved, as both organisms use a variant of the Min system to prevent polymerization of the tubulin-like protein FtsZ away from the mid-cell16,17. Both species also have a nucleoid occlusion system (Noc) inhibiting Z-ring formation over the chromosome to prevent ‘cutting’ of the chromosome during cell division18. Together, the Min and Noc systems ensure that cell division and septation occur when both sister chromatids have been fully replicated and segregated. These systems are, however, not conserved in all bacteria because the Gram-positive opportunistic human pathogen Streptococcus pneumoniae lacks homologues of the Min and Noc systems19. In contrast to E. coli and B. subtilis, the pneumococcal Z-ring forms readily over the nucleoid19,20. Recently, a pneumococcal-specific protein called RocS was identified that might fulfil a similar function to the Noc system by connecting chromosome segregation and capsule production21. Another S. pneumoniae-specific protein called MapZ was shown to guide Z-ring formation, analogous to the Min system in other bacteria22,23,24. Importantly, the position of the origin of replication (oriC) marks the approximate positions of future division sites25. In S. pneumoniae, cell division and DNA replication are thus intimately connected. However, it remains unknown how the cell senses when a new round of replication should be initiated.

We hypothesized that an unknown factor could be responsible for coordination of cell division and DNA replication in the pneumococcus. Using high-throughput gene silencing with clustered regularly interspaced short palindromic repeats interference (CRISPRi) of all essential genes of S. pneumoniae26, we examined proteins leading to defects in DNA content on depletion. Here, we describe the identification of Cell Cycle Regulator protein interacting with FtsZ (CcrZ), a conserved protein that activates DnaA to trigger initiation of DNA replication. Pneumococcal CcrZ localizes at the division site in a FtsZ-dependent manner and its inactivation leads to division defects. Together, our findings show that CcrZ acts as a spatiotemporal link between cell division and DNA replication in S. pneumoniae.

CcrZ is a conserved bacterial cell cycle protein

We previously generated a knockdown library using CRISPRi targeting 348 conditionally essential genes of the serotype 2 strain S. pneumoniae D39V that were identified by transposon-insertion sequencing26. Here, we investigated the function of spv_0476, encoding a protein of unknown function that is conserved in most Firmicutes (>30% identity) (Extended Data Fig. 1a). Silencing of spv_0476 by CRISPRi led to a drastic reduction in growth rate as well as the appearance of anucleate cells, as visualized by 4,6-diamidino-2-phenylindole (DAPI) staining (Fig. 1a,b). We renamed SPV_0476 as CcrZ for reasons explained below. ccrZ is in an operon with trmB, which encodes a transfer RNA methyltransferase and this operon structure is conserved across Firmicutes (Extended Data Fig. 1a). To exclude the possibility that the observed phenotypes of ccrZ silencing were caused by polar effects on trmB expression, we constructed a deletion of trmB. This deletion did not lead to growth defects (Extended Data Fig. 1b). Transposon-insertion sequencing indicated that ccrZ is essential26; however, we were able to generate a ΔccrZ deletion mutant, although cells grew slowly. We therefore constructed a depletion of CcrZ by ectopically expressing CcrZ under control of either an isopropyl-β-d-thiogalactoside (IPTG)- or a ZnCl2-inducible promoter (Plac and PZn respectively) and deleted ccrZ from its native location (ccrZ−/+ and PZnccrZ−/+ respectively). Depletion of CcrZ led to notable growth delay at 37 and 30 °C, confirming the CRISPRi observations (Extended Data Fig. 1b). Immunoblotting using a specific antibody raised against purified CcrZ confirmed depletion (Extended Data Fig. 1c).

Fig. 1: Depletion of CcrZ leads to anucleate cells and division defects.
figure1

a, Growth curve of cells with ccrZ targeted by CRISPRi (ccrZsgRNA + IPTG) indicates a clear growth defect when ccrZ is silenced. b, ccrZ silencing leads to the appearance of anucleate cells, as visualized by DAPI staining. Scale bar, 3 µm. c, ccrZ depletion by ectopic expression via the IPTG-inducible Plac promoter also leads to cells lacking a nucleoid, as observed by DAPI staining. Scale bar, 3 µm. d, Distribution of cell area of ccrZ-depleted cells, ccrZ depletion leads to a slight decrease in cell length and cell area. P = 1.5 × 10−27 and 3 × 10−22 when comparing length and area, respectively, values derived from two-sided Wilcoxon rank sum test. e, When a deletion of ccrZ is complemented (left), FtsZ–mTurquoise2 shows a clear mid-cell localization, whereas it appears as a blurry signal in several cells on ccrZ depletion (right). Scale bar, 3 µm. f, TEM indicates that cells depleted for ccrZ form multiple, often incomplete, septa. Scale bar, 250 nm. g, Distribution of number of septa per cell length as determined by TEM for n = 22 wild-type cells, n = 28 CcrZ-depleted cells and n = 17 CcrZ-complemented cells. Ratios are shown as box (25th to 75th percentile) and whisker (1.5× IQR) plots with individual data points overlaid as dot plots. P = 1 × 10−6 for wild-type versus ccrZ-depleted cells and P = 0.0013 for ccrZ-complemented versus ccrZ-depleted cells. P values were derived from a two-sided pairwise Wilcoxon rank sum test with Bonferroni adjustment.

Source data

In line with the CRISPRi observations, DNA staining of cells depleted for CcrZ showed that 20% of cells lacked a nucleoid (Fig. 1c, n = 442 cells counted). To test whether the ccrZ-deletion phenotype was conserved in other Gram-positive bacteria, we silenced ccrZ (SAOUHSC_01866, here ccrZSa) in Staphylococcus aureus SH1000 using CRISPRi and deleted the B. subtilis 168 ccrZ homologue (ytmP, here ccrZBs). Upon ccrZSa silencing in S. aureus, we observed a high proportion of anucleate cells, as well as a growth delay. By contrast, no anucleate cells were observed for B. subtilis (Extended Data Fig. 1d). However, cells deleted for ccrZBs were slightly thinner and longer, although they had a growth rate similar to wild-type cells (Extended Data Fig. 1d). Interestingly, S. pneumoniae ΔccrZ could not be complemented by expression of ccrZSa or ccrZBs. By contrast, depletion of S. aureus CcrZ was rescued by expression of CcrZBs (Extended Data Fig. 1d).

CcrZ depletion in S. pneumoniae also led to slight morphological defects and modest changes in cell size when analysed by phase-contrast microscopy (Fig. 1d). Polysaccharide capsule production has previously been linked to the pneumococcal cell cycle27, but capsule production was not impacted in a CcrZ mutant (Extended Data Fig. 1e). To visualize division sites in live cells, we constructed a translational fusion of mTurquoise2 to FtsZ (as the only copy of FtsZ, expressed from its native genetic location). As shown in Fig. 1e, Z-rings were clearly mislocalized upon CcrZ depletion for 3 h, with the presence of several aberrant Z-rings in 43% of the cells. To obtain further insight and verify that the increased number of septa are not due to the fluorescent protein fusion, we employed transmission electron microscopy (TEM) in untagged cells. Although not evident with phase-contrast microscopy, when ccrZ was depleted we observed frequent aberrant septum formation using TEM, and many cells harboured two (18%) to four (4%) septa, whereas only one septum is observed in 91% of wild-type cells (Fig. 1f,g).

S. pneumoniae CcrZ is part of the divisome

Because CcrZ seems to be involved in both chromosome biology and cell division, we examined its subcellular localization. Strikingly, immunofluorescence on fixed cells using a CcrZ-specific antibody demonstrated a mid-cell localization (Extended Data Fig. 2a). To assess the localization of CcrZ in live cells, we created functional fusions of a green fluorescent protein (GFP) to the N terminus of CcrZ (gfp–ccrZ) or a red fluorescent protein to the C terminus (ccrZ–mKate2) and inserted either construct at the native locus (Extended Data Fig. 1c). Epifluorescence microscopy of live bacteria showed that CcrZ localizes at mid-cell (Fig. 2a). This localization was conserved in both the TIGR4 and un-encapsulated R6 strains (Extended Data Fig. 2b). Interestingly, CcrZSa and CcrZBs did not localize as clear rings at mid-cell in S. aureus and B. subtilis (Extended Data Fig. 2b), indicating that activity and/or localization of CcrZ in these organisms is regulated differently. To obtain higher spatial resolution of S. pneumoniae GFP–CcrZ, 240 images (16 stacks) on live cells were acquired using three-dimensional structured illumination microscopy (3D-SIM) and reconstructed to generate a super-resolution image. As shown in Fig. 2b and Supplementary Video 1, CcrZ forms a patchy ring at mid-cell. Furthermore, time-lapse microscopy showed that CcrZ disassembles from the old septum to assemble at the newly formed division site (Supplementary Video 2).

Fig. 2: CcrZ colocalizes with FtsZ at new division sites.
figure2

a, CcrZ localizes at mid-cell in live wild-type S. pneumoniae cells as observed by epifluorescence microscopy of GFP–CcrZ and CcrZ–mKate2. Scale bar, 3 µm. b, 3D-SIM of GFP–CcrZ and reconstructed volume projection (right) indicate that CcrZ forms a patchy ring at the mid-cell. Scale bar, 2 µm (left and middle right); 500 nm (right). c, GFP–CcrZ and FtsZ–mCherry colocalize in wild-type cells. Scale bar, 3 µm. d, Localization signal of GFP–CcrZ and FtsZ–mCherry in n = 699 cells of a double-labelled gfp–ccrZ ftsZ–mCherry strain, ordered by cell length and represented by a heatmap. e, GFP–CcrZ and FtsZ–mCherry colocalize during the entire cell cycle, as visualized when signal localization over cell length is grouped in three quantiles. f, 3D-SIM colocalization of GFP–CcrZ and FtsZ–mCherry shows a clear colocalizing ring with an identical patchy pattern. Note that for clarity, we did not correct for chromatic shift in the overlay. Scale bar, 2 µm.

Source data

To test whether the mid-cell localization of S. pneumoniae CcrZ coincides with FtsZ, we constructed a double-labelled strain (gfp–ccrZ ftsZ–mCherry). As shown in Fig. 2c, CcrZ colocalized with FtsZ (Fig. 2c–e and Supplementary Video 3). Note that the FtsZ–mCherry fusion did not affect growth or morphology28. 3D-SIM also showed a similar colocalizing pattern (Fig. 2f, Extended Data Fig. 2c and Supplementary Video 4).

Prediction of CcrZ’s topology using TMHMM29 did not indicate the presence of a transmembrane domain; the septal localization of CcrZ might then rely on another partner. To identify possible partners, we purified GFP–CcrZ expressed from S. pneumoniae and untagged cytosolic superfolder GFP as a control using anti-GFP nanobodies without cross-linking, and directly analysed the purified fraction using liquid chromatography tandem mass spectrometry. Interestingly, we found an enrichment (more than fivefold change) for several proteins from the divisome (for example, FtsZ, PBP2X and EzrA) (Supplementary Table 3). To determine which of the candidates might interact directly with CcrZ, we used the NanoBit complementation reporter assay30,31, which uses a luciferase separated into a large bit (LgBit) and a small bit (SmBit). Fusion of two different interacting proteins to each fragment can restore the activity of the luciferase and, in the presence of a furimazine-based substrate, produce light30. Accordingly, we fused the C-terminal extremity of CcrZ to LgBit and putative partners to SmBit and integrated the different constructs at their respective loci under native control. We also fused SmBit to other proteins known to localize at the septum (Cps2E, FtsA, FtsW and ZapA). We used a strain expressing both HlpA–LgBit and HlpA–SmBit as a positive control for interaction30. After addition of substrate, we could detect a strong signal between FtsZ and CcrZ, as well as a weaker signal for FtsA, EzrA and ZapA, and no detectable signal for any of the other proteins (Fig. 3a). This result indicates that FtsZ and CcrZ in S. pneumoniae are in very close proximity in space. Interestingly, a weak signal was also observed for CcrZ–LgBit and CcrZ–SmBit (Fig. 3a).

Fig. 3: CcrZ interacts directly with FtsZ.
figure3

a, Split-luciferase assay using several combinations with CcrZ–LgBit reveals that CcrZ and FtsZ are in very close proximity, as indicated by a high luminescence signal. FtsA, EzrA and ZapA, all three interacting directly with FtsZ, also gave a slight signal. hlpA–LgBit hlpA–SmBit (HlpA–HlpA), here diluted 100 times, is used as a positive control. Each dot represents the average of n = 15 measurements of a technical replicate, with the size of the dot representing the s.e.m. RLU, relative luminescence units. b, FtsZ–CcrZ interaction confirmation by bacterial two-hybrid assay. T25 is the empty vector pST25 and T25–FtsZ corresponds to vector pST25–FtsZ used in combination with pUT18–CcrZ (CcrZ–T18) and pUT18–FtsZ (FtsZ–T18). c, Affinity purification of FtsZ–GFP from S. pneumoniae cells (second lane) also pulls down untagged CcrZ (fourth lane). Purification of GFP alone (first lane) did not pull-down CcrZ (third lane). d, FtsZ from S. pneumoniae expressed in E. coli copurifies with CcrZSp–GFP by affinity purification. WC, whole-cell extract; S, supernatant; HE, heat-eluted products; C, CcrZ–GFP; F, FtsZ. e, Epifluorescence time-lapse microscopy of CcrZ–mKate2 at 37 °C in the presence (left) or absence (right) of FtsZ. When FtsZ amounts are reduced, cells increase their size and CcrZ is delocalized from the mid-cell. Scale bar, 3 µm.

Source data

To confirm the observed interaction with FtsZ, we used a bacterial two-hybrid assay in E. coli32. Again, we observed a robust interaction between CcrZ and FtsZ (Fig. 3b). Co-immunoprecipitation of FtsZ–GFP from S. pneumoniae cells confirmed the in vivo interaction with CcrZ (Fig. 3c). Affinity purification of CcrZSp–GFP when overexpressing FtsZSp in E. coli also confirmed this interaction because we were able to copurify FtsZ (Fig. 3d). To test whether the localization of CcrZ depends on FtsZ, we constructed a strain expressing CcrZ–mKate2 as well as a second copy of FtsZ under the control of an IPTG-inducible promoter and deleted the native ftsZ gene (ftsZ−/+). As expected, FtsZ depletion led to aberrant cell morphology and CcrZ–mKate2 was rapidly mislocalized (Fig. 3e and Supplementary Video 5). We conclude that CcrZ localizes to new division sites via a direct interaction with FtsZ.

CcrZ controls DNA replication

To investigate the consequences of a lack of CcrZ on chromosome segregation in live cells, we introduced a translational fluorescent fusion of HlpA33 and deleted ccrZ. Localization of HlpA–mKate2 in this slow-growing ΔccrZ mutant showed similar results to DAPI-stained cells depleted for CcrZ and we observed that 19% of cells lacked a nucleoid signal (Extended Data Fig. 3a; 4,855 cells counted). Time-lapse imaging indicated that cells with defective DNA content had either no DNA at all or chromosomes ‘guillotined’ during septum closure suggesting reduced nucleoid occlusion control (Fig. 4a and Supplementary Video 6). We also colocalized FtsZ fused to a cyan fluorescent protein (FtsZ–CFP) with HlpA–mKate2 while depleting CcrZ for a short time (2 h). Interestingly, we observed many cells with a chromosome localized at only one half of the cell (Fig. 4b).

Fig. 4: CcrZ-depleted cells under replicate.
figure4

a, Time-lapse microscopy of HlpA–mKate2 at 30 °C in a ΔccrZ mutant. Orange arrows indicate cells with no nucleoid; white arrows indicate cells with ‘guillotined’ DNA. b, FtsZ–CFP and HlpA–mKate2 colocalization on ccrZ depletion. c, Growth of three ccrZ suppressor mutants (ccrZsupp1−3) compared with ccrZ depletion (orange). d, DAPI staining of the three suppressor mutants. e, Schematic representation of the suppressor mutations within DnaA domain III and within the YabA DnaA/DnaN binding motif (ANB). TM, tetramerization domain. f,g,i,j,l,o, oriC/ter ratios determined by RT–qPCR. Mean values are indicated under the boxes. Data from Monte Carlo simulations (Methods) are shown as box (25th to 75th percentile) and whisker (1.5× IQR) plots with outliers as dots. *P < 0.05, values calculated by bootstrap. f, oriC/ter ratios for D39V wild-type and ccrZ depleted cells; n = 3 independent samples. g, oriC/ter ratios for S. aureus on ccrZSa depletion; n = 4 independent samples. h, oriC/ter ratios on ccrZBs deletion in B. subtilis as determined by RT–qPCR. Mean values are indicated under the boxes. Data are shown as box (25th to 75th percentile) and whisker (1.5× IQR) plots. *P = 0.02 two-sided t-test; n = 3 independent samples. i, oriC/ter ratios of ΔccrZ with dnaA suppressor mutations; n = 3 independent samples. j, oriC/ter ratios of ∆yabA ΔccrZ and ΔccrZ yabA-E93*; n = 3 independent samples. k, Growth of ΔyabA ΔccrZ and ΔccrZ dnaA-Q247H/S292G compared with ccrZ depletion. l, oriC/ter ratios of dnaA-Q247H and dnaA-S292G in a wild-type background. m, Schematic overview of CRISPRi-seq. A library expressing 1,499 different sgRNAs targeting 2,111 genetic elements was grown while expressing or repressing dCas9. sgRNA counts after Illumina sequencing indicate which operons become more (beneficial) or less (detrimental) essential in a ccrZ depletion background. n, CRISPRi-seq of ccrZ depletion versus ccrZ expression shows a positive interaction between ccrZ and yabA/holB and a negative interaction between ccrZ and ftsK/rocS. o, oriC/ter ratios for FtsZ depletion (−IPTG) and complementation (+IPTG); n = 12 independent samples. Scale bars, 3 µm.

Source data

When attempting to make clean ccrZ deletions, in addition to small colonies typical of slow-growing mutants, there were also spontaneous large, wild-type sized colonies. Growth analysis of three of these large colonies (ccrZsupp1–3) showed that cells behaved like wild-types, and DAPI staining revealed normal DNA content (Fig. 4c,d). To verify whether these wild-type-like phenotypes were caused by suppressor mutations, we performed whole genome sequencing. All three strains still contained the ccrZ deletion and a single nucleotide polymorphism (Fig. 4e). Two missense mutations were found in dnaA (DnaA-Q247H and DnaA-S292G) and one nonsense mutation in yabA (YabA-E93*). Because DnaA promotes initiation of DNA replication and YabA hampers it by preventing interaction of DnaA with DnaN34, we wondered whether the frequency of DNA replication initiation was changed in a ccrZ mutant.

To test this hypothesis, we quantified the copy-number ratio between chromosomal origin and terminus regions (oriC/ter ratios) using a real-time quantitative polymerase chain reaction (RT–qPCR). In a wild-type situation, during exponential growth, the oriC/ter ratio varies between 1.3 and 1.8, because most cells have started a round of replication (note that in contrast to E. coli and B. subtilis, multifork replication does not occur in S. pneumoniae)35. Remarkably, depletion of CcrZ resulted in a significantly decreased DNA replication initiation rate with an oriC/ter ratio of 1.1 versus 1.8 for complemented cells (P < 0.05) (Fig. 4f). Interestingly, the same observation was made for both B. subtilis and Staphylococcus aureus, where deletion or depletion of CcrZ caused a clear reduction in oriC/ter ratios (Fig. 4g,h). Because the identified ccrZ-bypass mutations were found in DNA replication initiation regulators, we tested whether they would restore the oriC/ter ratio in a fresh ccrZ deletion background in S. pneumoniae. Indeed, the oriC/ter ratios for ΔccrZ dnaA-S292G, ΔccrZ dnaA-Q247H and yabA-E93* (ccrZsupp3) were like wild-type (Fig. 4i,j).

The point mutation found in yabA causes premature translation termination at the C terminus of YabA. When yabA alone was replaced by an antibiotic resistance cassette, we observed an increase in replication initiation as well as a reduced growth rate; but when ccrZ was codeleted, wild-type-like growth and oriC/ter ratio was observed (Fig. 4j,k). DnaA suppressor mutations were located in the AAA+ ATPase domain of DnaA36 (Extended Data Fig. 3b) and it was previously reported that specific mutations in this domain could increase the initiation rate in B. subtilis37. To determine whether those mutations alone were able to induce overinitiation, we inserted each dnaA mutation into a wild-type background. Marker frequency analysis detected an increase in the oriC/ter ratio for both dnaA alleles (Fig. 4l). We conclude that mutations that increase the rate of initiation of DNA replication can rescue the ∆ccrZ phenotype.

To gain additional insights into CcrZ function, we performed a genome-wide genetic interaction screen using CRISPRi-seq38 (Fig. 4m). This technique relies on the expression of dCas9, controlled by an anhydrotetracycline (aTc)-inducible promoter, and constitutive expression of a specific single guide RNA (sgRNA) that together form a roadblock for the RNA polymerase and thereby downregulate transcription of the targeted operon. We created a CRISPRi library by transforming S. pneumoniae Ptet–dCas9, Plac–ccrZ, ∆ccrZ with 1,499 different sgRNAs targeting 2,111 of 2,146 genetic elements of S. pneumoniae. The resulting library was grown in the presence or absence of aTc/IPTG and the sgRNAs were Illumina sequenced. After analysing the fold change for every sgRNA between ccrZ-depletion and ccrZ-complementation, we found an enrichment of sgRNAs targeting the operon of YabA/HolB (tmk-holB-yabA-spv_0828), confirming that depletion of YabA can complement ∆ccrZ (Fig. 4n and Supplementary Table 4). Interestingly, we also found that inactivation of ftsK and rocS worsened the fitness of a ccrZ mutant. RocS is a regulator of chromosome segregation21 and FtsK is important for chromosome segregation during cell division39. These interactions reinforce a role of CcrZ in chromosome integrity and replication and that CcrZ acts in a distinct pathway from these chromosome segregation factors. Finally, to test whether the mid-cell localization of CcrZ is important for well-timed replication of the chromosome, we abrogated CcrZ’s mid-cell localization by depleting cells for FtsZ (Fig. 3e). After 2 h of FtsZ depletion, chromosomal DNA was isolated and oriC/ter ratios were determined. This showed that on mis-localization of CcrZ, cells under-replicate (Fig. 4o).

CcrZ is a conserved regulator of DnaA

The results so far suggest that the division defects observed in the absence of CcrZ are caused by under-replication of the chromosome. To examine whether disruption of DNA replication in general could lead to defects in division, we took advantage of a thermosensitive dnaA mutant (dnaATS) in which DNA replication initiation is reduced when cells are grown at a non-permissive temperature (40 °C)21. As expected, when shifted to the non-permissive temperature, many cells were anucleate (Extended Data Fig. 4a). Strikingly, localization of FtsZ–mTurquoise2 in the dnaATS strain at 40 °C phenocopied the ∆ccrZ mutant, and FtsZ was frequently mislocalized (Fig. 5a). Examination by time-lapse microscopy following a temperature shift from 30 °C to 40 °C showed that FtsZ–mTurquoise2 mis-localization occurs after four to five generations (Supplementary Video 7). Furthermore, examination by TEM at 40 °C showed many cells with aberrant septa (Fig. 5b). These data are consistent with the idea that CcrZ exerts a control on DNA replication initiation.

Fig. 5: CcrZ activates DnaA-dependent replication initiation.
figure5

a, Localization of FtsZ–mTurquoise2 in a thermosensitive DnaA strain (dnaATS) at permissive (30 °C) and non-permissive (40 °C) temperatures shows that dnaA inactivation leads to a similar phenotype as ccrZ inactivation. Scale bar, 3 µm. b, TEM of DnaATS at a non-permissive temperature (40 °C) indicates the presence of multiple septa, similar to a ΔccrZ mutant. Scale bar, 250 nm. c, When replication is driven in a RepN-dependent manner in B. subtilis (oriN), no decrease in ori/ter ratio can be observed in the absence of ccrZBs (oriN, ΔccrZBs). Mean values are indicated under the boxes. Data are shown as box (25th to 75th percentile) and whisker (1.5× IQR) plots; n = 3 independent samples. d, Schematic representation of CcrZ motifs. CcrZ has one putative domain annotated APH (phosphotransferase enzyme family; PFAM01636). Sequence alignment with several kinases revealed the presence of a conserved P-loop, APH and Brenner’s motifs, found in most phosphotransferases. Locations of mutations made for three essential (red) and two non-essential (black) conserved residues are shown underneath. e, LicA choline kinase structure complexed with AMP and MES buffer. The five residues indicated in yellow are conserved between CcrZ and LicA (and highly conserved within Firmicutes). f, Mutation of three of these five conserved residues in the putative ATP-binding pocket leads to growth defects. g, Localization of CcrZ–H157A–GFP and CcrZ–D177A–GFP is not impaired. Scale bar, 3 µm.

Source data

To test whether CcrZ controls DNA replication by regulating DnaA activity, we made use of the fact that a B. subtilisccrZBs mutant also underinitiates (Fig. 4h) and a strain was constructed in which DNA replication was driven in a RepN-dependent manner (from a plasmid origin of replication oriN) rather than from DnaA-dependent initiation (from oriC). This showed no significant ori/ter ratio differences when ccrZ was deleted (Fig. 5c), suggesting that CcrZ is an activator of DnaA-dependent initiation of replication in B. subtilis. We tested whether CcrZ interacts directly with DnaA and employed bacterial two-hybrid assays and the Split-luc system using pneumococcal CcrZ and DnaA (Fig. 3a and Extended Data Fig. 4b). However, none of these assays revealed a direct protein–protein interaction. Also, in line with our genetic data, we did not find a direct interaction of CcrZ with YabA, although YabA interacts with DnaA (Extended Data Fig. 4c). It is still possible that CcrZ interacts directly with DnaA, but that we cannot detect it with these assays. Alternatively, another factor might be required for CcrZ’s function or CcrZ indirectly affects the activity of DnaA.

CcrZ’s conserved residues are essential for its function

S. pneumoniae CcrZ is predicted to have a single aminoglycoside phosphotransferase enzyme family (APH) domain (Fig. 5d). Pairwise comparisons of profile-hidden Markov models (HMMs) using HHpred40 identified homologies with ethanolamine and choline kinases. Because CcrZ is highly conserved in Firmicutes, we aligned CcrZ with 1,000 sequences from UniRef50 and identified three residues conserved in more than 95% of the proteins (D159, N164 and D177) and two other residues (H157 and D189) conserved in more than 80% (Fig. 5d and Extended Data Fig. 4d). To determine the position of these residues, CcrZ was mapped onto the crystal structure of the best hit from the HMM alignment, the choline kinase LicA, in complex with adenosine monophosphate (AMP) (pdb 4R78). Interestingly, the five conserved residues are in spatial proximity to AMP (Fig. 5e). Comparison of CcrZ and LicA shows a conserved Brenner’s motif [HXDhX3N] (residues CcrZ H157–N164) found in most phosphotransferases (Fig. 5d). In this motif, LicA–N187 (CcrZ–N164) was shown to interact with the α-phosphate moiety of AMP41 and LicA–D176 (CcrZ–D159) was shown to be crucial for hydrogen bond formation with the hydroxyl moiety of choline. LicA–D194 (CcrZ–D177) interacts with the α-phosphate moiety of AMP. CcrZ, however, does not possess the conserved hydrophobic residues specific to choline and ethanolamine kinases necessary for choline binding, but instead has several polar amino acids at these positions. Mutational analysis of the five conserved residues of CcrZ showed that at least H157, N164 and D177 are essential for CcrZ’s function in S. pneumoniae (Fig. 5f), while mutating CcrZ–D159 or CcrZ–D189 did not lead to growth defects. All three essential mutants were properly produced (Extended Data Fig. 1c) and CcrZ–H157A and CcrZ–D177A could still localize at the septum (Fig. 5g). Given the high similarity with LicA, it is very likely that CcrZ can bind an as yet unknown nucleotide.

A model for CcrZ-controlled DNA replication in S. pneumoniae

In S. pneumoniae, once DNA replication initiates at the mid-cell, the origins localize at both future division sites, while the replication machinery stays near the Z-ring until completion of replication and closure of the septum25. We therefore hypothesized that CcrZ is brought to the mid-cell by FtsZ to promote initiation of DNA replication. To map the hierarchy of events that take place during the pneumococcal cell cycle, we constructed a triple-labelled strain (strain ccrZ–mKate2 dnaN–sfTQOX parBp–mYFP) in which CcrZ is fused to a red fluorescent protein, DNA replication is visualized by DnaN fusion to a cyan fluorescent protein and the origin of replication is marked with a yellow fluorescent reporter. Imaging using time-lapse fluorescence microscopy revealed that DNA replication initiates once CcrZ is assembled at the mid-cell, rapidly followed by segregation of the newly replicated origins as cells elongate (Fig. 6a–d and Supplementary Video 8). The replication machinery remains near the old division site together with CcrZ, moving to the new cell division sites only once DNA replication is complete. These data support a model in which FtsZ brings CcrZ to oriC to stimulate DnaA to fire a new round of replication ensuring that DNA replication commences only after the origins are well segregated and positioned at the new mid-cell position. Indeed, DnaA colocalizes with CcrZ in newborn cells (Extended Data Fig. 5). In the absence of CcrZ, initiation of DNA replication is mis-timed and occurs too late relative to cellular growth and Z-ring formation, frequently leading to futile division events, mis-segregated chromosomes and anucleate cells (Fig. 6e).

Fig. 6: Spatiotemporal localization of CcrZ via FtsZ ensures proper timing of DNA replication in S. pneumoniae.
figure6

a, Microscopy of the origin of replication (yellow), replication fork (cyan) and CcrZ (red) in live S. pneumoniae wild-type background cells. Scale bar, 1 µm. b, DnaN, oriC and CcrZ localizations grouped by cell area (µm2) in five equally sized groups. Analysed from snapshots of exponentially growing cells. c, Single-cell kymographs of DnaN, CcrZ and oriC localizations in a 2:30 minute interval time-lapse video. d, Tracked DnaN, oriC and CcrZ over time in a single cell. Top: overlay of fluorescence, cell outline and phase-contrast of the cell displayed in panel c. Bottom: fluorescence localization on the length axis of the same single cell over time. e, Model for spatiotemporal control of replication by CcrZ. In S. pneumoniae, CcrZ is brought to the middle of the cell where the DnaA-bound origin of replication is already positioned. CcrZ then stimulates DnaA to trigger DNA replication by an as yet unknown activity, possibly involving a phosphor-transfer event. Whereas the precise regulation and localization of CcrZ seems diverse between different organisms, CcrZ’s activity to stimulate DNA replication is conserved, at least in S. pneumoniae, S. aureus and B. subtilis.

Source data

Discussion

The principal contribution of this work is the identification and initial functional characterization of a mechanism for cell cycle regulation in S. pneumoniae via CcrZ. We show that CcrZ’s septal localization occurs via direct interaction with FtsZ. Our data are consistent with a model in which, once positioned at mid-cell, CcrZ stimulates DnaA, probably by phosphorylation of an intermediate molecule, to initiate DNA replication (Fig. 6). Importantly, CcrZ’s function of controlling DnaA seems conserved in S. aureus and B. subtilis, and probably in many other Gram-positive bacteria (Extended data Fig. 1a). In some ways, CcrZ resembles MipZ of Caulobacter crescentus in terms of one protein coordinating several aspects of the cell cycle. Whereas CcrZ stimulates replication after division has taken place, MipZ positions the Z-ring and delays division until chromosome segregation has initiated42.

Besides the production of anucleate cells and cells with cleaved chromosomes, ccrZ mutants contain multiple aberrant division septa (Fig. 6e). Notably, this is phenocopied by a temperature-sensitive DnaA allele. This indicates that chromosome replication itself, and correct localization of the chromosome has an important role in nucleoid occlusion: when initiation is too late and the new daughter chromosomes are not fully segregated, division can take place over the DNA resulting in dissected chromosomes. We also observed multiple division septa in cells depleted for CcrZ that are probably caused by mis-timed chromosome segregation, whereby Z-rings are formed adjacent to the nucleoid. These phenotypes are reminiscent of observations made for E. coli and B. subtilis that showed that after arrest of DNA replication, many cells continued to elongate without dividing, but Z-rings continued to form to the side of nucleoids43,44. It is interesting to note that the Staphylococcus aureus Noc system also controls DNA replication, because Δnoc cells overinitiate DNA replication45. A lethal S. aureus Δnoc ΔcomEB double mutant could be rescued by a suppressor mutation in ccrZSa45, further supporting that CcrZSa is also involved in the control of DNA replication.

This work uncovers a mechanism in which a single protein links cell division with DNA replication control. In this model, Z-ring formation is used as a timer for the initiation of DNA replication. When cell division terminates, leading to the formation of another Z-ring at the new division site, CcrZ is brought along and can activate a new round of DNA replication. This simple system ensures that DNA replication commences only once per cell cycle. It will be interesting to see how CcrZ controls the cell cycle in other bacteria, what the involved biochemical activities are and whether CcrZ will prove a new target for innovative antibiotics.

Methods

Bacterial strains and culture conditions

All strains, plasmids and primers used are listed in Supplementary Table 1 and Supplementary Table 2.

All pneumococcal strains in this study are derivates of S. pneumoniae D39V46, unless specified otherwise, and are listed in Supplementary Table 1. Strains were grown in liquid semidefined C+Y medium47 at 37 °C from a starting optical density (OD600) of 0.01 until the appropriate OD. Induction of the zinc-inducible promoter (PZn) was carried out by supplementing the medium with 0.1 mM ZnCl2 and 0.01 mM MnCl2 (Sigma-Aldrich) and the IPTG-inducible promoter (Plac) was activated with 1 mM IPTG (Sigma-Aldrich). For all related experiments, depletion strains were first grown without inducer until OD600 = 0.3 and then diluted 100 times in fresh medium and grown until the desired OD. Transformation of S. pneumoniae was performed as described previously47 with cells taken at the exponential growth phase (OD600 = 0.1). When necessary, the medium was supplemented with the following antibiotics: chloramphenicol (0.45 µg ml−1), erythromycin (0.2 µg ml−1), kanamycin (250 µg ml−1), spectinomycin (200 µg ml−1) and tetracycline (0.5 µg ml−1).

Staphylococcus aureus strains are listed in Supplementary Table 1. Cells were grown in brain heart infusion medium (Oxoid) with shaking at 37 °C. When appropriate, 5 µg ml−1 of erythromycin and/or 10 µg ml−1 of chloramphenicol was added to the growth medium. All Staphylococcus aureus plasmids were initially made in E. coli strain IM08B48. E. coli IM08B was grown in Luria–Bertani (LB) medium at 37 °C with shaking; 100 µg ml−1 of ampicillin was added when appropriate. Plasmids were then transformed into S. aureus by electroporation, as described previously49.

B. subtilis strains are listed in Supplementary Table 1. Cells were grown with shaking at 37 °C in LB medium or S7 defined minimal medium with MOPS buffer at a concentration of 50 mM rather than 100 mM supplemented with 1% glucose, 0.1% glutamate, trace metals, 40 μg ml−1 phenylalanine and 40 μg ml−1 tryptophan50. Standard concentrations of antibiotics were used when appropriate. B. subtilis strains were derived from 1A700 or JH642 (pheA1 trpC2)51.

Strain construction

Construction of strains is described in the Supplementary Methods.

Microtitre plate-based growth assay

For S. pneumoniae growth assays, cells were first grown in C+Y medium pH 7.4 until the mid-exponential growth phase (OD595 = 0.3) with no inducer at 37 °C, after which they were diluted 100 times in fresh C+Y medium supplemented with IPTG or ZnCl2 when appropriate. Cellular growth was then monitored every 10 min at either 37 °C or 30 °C in a microtitre plate reader (TECAN Infinite F200 Pro). Each growth assay was performed in triplicate. The lowest OD595 of each growth curve was normalized to 0.004 (detection limit of the reader and initial OD595 of the inoculum) and the average of the triplicate values were plotted, with the s.e.m. represented by an area around the curve.

For assessment of S. aureus growth, CRISPRi knockdown strains were grown overnight in brain heart infusion medium. Cultures were then diluted 100-fold and grown until OD600 = 0.4. The cultures were then re-diluted 200-fold in medium with or without inducer 500 µM IPTG. Growth analysis was performed on a Synergy H1 Hybrid (BioTek) microtiter plate reader at 37 °C with measurement of OD600 every 10 min. The averages of the triplicate values were plotted, with the s.e.m. represented by an area around the curve.

Phase-contrast and fluorescence microscopy

S. pneumoniae cells were grown in C+Y medium pH 7.4 at 37 °C to an OD595 = 0.1 without any inducer and diluted 100 times in fresh C+Y medium supplemented when appropriate with IPTG (for activation of dCas9, complementation of CcrZ and FtsZ, or expression of fluorescent fusions) or ZnCl2 (for CcrZ complementation or expression of fluorescent fusions). At OD595 = 0.1, 1 ml of culture was harvested by centrifugation for 1 min at 9,000g. For DAPI staining, 1 µg ml−1 of DAPI (Sigma-Aldrich) was added to the cells and incubated for 5 min at room temperature before centrifugation. For imaging of bulk exponentially growing cultures, cells were washed twice with 1 ml of ice-cold PBS and resuspended in 50 µl of ice-cold PBS; for time-lapse microscopy, cells were washed and resuspended in 1 ml of fresh prewarmed C+Y medium. One microlitre of cells were then spotted onto PBS- or C+Y-polyacrylamide (10%) pads. For time-lapse microscopy, pads were incubated twice for 30 min in fresh C+Y medium at 37 °C before spotting. Pads were then placed inside a gene frame (Thermo Fisher Scientific) and sealed with a cover glass as described previously52. Microscopy acquisition was performed using either a Leica DMi8 microscope with a sCMOS DFC9000 (Leica) camera and a SOLA light engine (Lumencor) or a DV Elite microscope (GE Healthcare) with a sCMOS (PCO-edge) camera and a DV Trulight solid-state illumination module (GE Healthcare), and a ×100/1.40 oil-immersion objective. Phase-contrast images were acquired using transmission light (100 ms exposure). Still fluorescence images were usually acquired with 700 ms exposure, and time-lapses with 200–300 ms exposure. The Leica DMi8 filters set used were as followed: DAPI (Leica 11533333, Ex: 395/25 nm, BS: LP 425 nm, Em: BP 460/50 nm), CFP (Ex: 430/24 nm Chroma ET430/24x, BS: LP 455 Leica 11536022, Em: 470/24 nm Chroma ET470/24 m), GFP (Ex: 470/40 nm Chroma ET470/40x, BS: LP 498 Leica 11536022, Em: 520/40 nm Chroma ET520/40 m), yellow fluorescent protein (YFP) (Ex: 500/20 nm Chroma ET500/20x, BS: LP 520 Leica 11536022, Em: 535/30 nm Chroma ET535/30 m) and mCherry (Chroma 49017, Ex: 560/40 nm, BS: LP 590 nm, Em: LP 590 nm). DeltaVision microscope used a DV Quad-mCherry filter set: GFP (Ex: 475/28 nm, BS: 525/80 nm, Em: 523/36 nm) and mCherry (Ex: 575/25 nm, BS: 605/50, Em: 632/60 nm). Images were processed using either LasX v.3.4.2.18368 (Leica) or SoftWoRx v.7.0.0 (GE Healthcare). For Staphylococcus aureus microscopy, cells were induced as described above, grown until OD600 = 0.2 and analysed on a Zeiss AxioObserver with an ORCA‐Flash4.0 V2 Digital CMOS camera (Hamamatsu Photonics) through a ×100 PC objective. An HPX 120 Illuminator (Zeiss) was used as a light source for fluorescence microscopy. Images were processed using ZEN Blue v.1.1.2.0 (Zeiss). Signals was deconvolved, when appropriate, using Huygens v.17.10.0p4 (SVI) software.

Transmission electron microscopy

Strains were grown in C+Y medium at either 37 °C, or at 30 °C for dnaATS, until OD595 = 0.3, with or without addition of ZnCl2 (for ccrZ complementation or depletion, respectively) and diluted 100 times in 10 ml of fresh C+Y medium. Cells were then grown at either 37 °C or 40 °C, for dnaA depletion in the dnaATS strain, until OD595 = 0.15. Five millilitres of each sample was then fixed with 2.5% glutaraldehyde solution (EMS) in phosphate buffer (PB 0.1 M pH 7.4) (Sigma-Aldrich) for 1 h at room temperature, followed by 16 h incubation at 4 °C. Cells were then postfixed using a fresh mixture of osmium tetroxide 1% (EMS) with 1.5% potassium ferrocyanide (Sigma-Aldrich) in PB for 2 h at room temperature. Samples were then washed three times with distilled water and spun down in low-melting agarose 2% (Sigma-Aldrich) and solidified in ice. Solid samples were cut in 1-mm3 cubes and dehydrated in acetone solution (Sigma-Aldrich) at graded concentrations (30% for 40 min; 50% for 40 min; 70% for 40 min and 100% for 3 × 1 h). This step was followed by infiltration in Epon (Sigma-Aldrich) at graded concentrations (Epon 1/3 acetone for 2 h; Epon 3/1 acetone for 2 h, Epon 1/1 for 4 h and Epon 1/1 for 12 h) and finally polymerized for 48 h at 60 °C. Ultra-thin sections of 50 nm were then cut on a Leica Ultracut (Leica Mikrosysteme) and placed on a copper slot grid 2 × 1 mm (EMS) coated with a polystyrene film (Sigma-Aldrich). Sections were subsequently poststained with 4% uranyl acetate (Sigma-Aldrich) for 10 min, rinsed several times with water, then with Reynolds lead citrate (Sigma-Aldrich) for 10 min and rinsed several times with distilled water. Micrographs were taken using a transmission electron microscope Philips CM100 (Thermo Fisher Scientific) equipped with a TVIPS TemCam-F416 digital camera (TVIPS) and using an acceleration voltage of 80 kV. Number of septa and cell length were measured manually on TEM images of cells in the correct focal plane: n = 22 wild-type cells, n = 28 ccrZ-depleted cells and n = 17 ccrZ-complemented cells.

3D-structured illumination microscopy

Samples for 3D-SIM were prepared as described previously by spotting 1 µl onto PBS–10% acrylamide pads. Acquisition was performed on a DeltaVision OMX SR microscope (GE Healthcare) equipped with a ×60/1.42 NA objective (Olympus) and 488 nm and 568 nm excitation lasers. Sixteen Z-sections of 0.125 μm each were acquired in Structure Illumination mode with 20 ms exposure and 20% laser power. The 240 images obtained were reconstructed with a Wiener constant of 0.01, and the volume reconstructed using SoftWoRx.

Image analysis and cells segmentation

All microscopy images were processed using FIJI v.1.52q (fiji.sc). Cell segmentation based on phase-contrast images was performed using either Oufti53, MicrobeJ54 or Morphometrics55 and fluorescent signals where analysed using Oufti (for CcrZ and FtsZ), MicrobeJ54 (for CcrZ) or iSBatch56 (for DnaN and oriC). Fluorescence heat-maps were generated using BactMAP57.

Small-scale expression and GFP resin pull-down of FtsZ and CcrZ–GFP

For affinity purification of CcrZSp–GFP while expressing FtsZSp, ccrZSp was amplified from D39V genomic DNA with primers 213/214 and the resulting fragment was assembled using Golden Gate allelic replacement strategy (BsaI) with plasmid pET-Gate2 ccdB (pSG436), pSG366, pSG367 and pSG2562, resulting in plasmid pSG2950. ftsZ was amplified by PCR 215/216 on D39V genomic DNA and cloned into plasmid pJet1.2, resulting in plasmid pSG4227. The latter was then assembled with pSG1694 using Golden Gate assembly, leading to plasmid pSG4268. BL21 DE3 Gold competent cells were cotransformed with plasmids containing one each of S. pneumoniae FtsZ and CcrZ–GFP. Expression was ZYM-5052 autoinduction media58. Cells were sonicated in buffer containing 50 mM Tris pH 7.5, 150 mM potassium acetate, 5% glycerol and 5 mM β-mercaptoethanol (lysis buffer). Supernatant was then mixed with GFP resin which was produced by cross-linking nanobody59 to NHS-Activated Sepharose 4 Fast Flow beads (GE Healthcare) according to the manufacturer’s instructions. After 1 h of batch binding, resin was washed 10 column volume (CV) with lysis buffer. Beads were then resuspended in 50 µl of lysis buffer mixed with SDS–PAGE loading dye containing 5% w/v β-mercaptoethanol and heat treated at 95 °C for 15 min. Supernatant was collected and labelled heat elution samples. Whole-cell lysate, supernatant after sonication, and heat elution samples were loaded onto 15% SDS–PAGE gels and visualized by Coomassie staining.

Large-scale purification of CcrZ–CPD for antibody production

To express a fusion of S. pneumoniae CcrZ with a C-terminal cysteine protease domain, ccrZ was amplified by PCR from D39V genomic DNA with primers 213/214 and assembled using Golden Gate allelic replacement strategy (BsaI) with plasmid pET-Gate2 ccdB (pSG436), pSG366, pSG367 and pSG2559. The resulting pSG2949 plasmid was then transformed into BL21 DE3 Gold cells using ZYM-5052 autoinduction media58. Cells were sonicated in buffer containing 300 mM NaCl, 50 mM Tris pH 7.5, 5 mM β-mercaptoethanol and protease inhibitor cocktail. Supernatant was loaded onto a gravity flow column containing HisPur Cobalt Resin (Thermo Scientific). The column was washed 5 CV with buffer containing 100 mM NaCl, 20 mM Tris pH 7.5 and 5 mM β-mercaptoethanol. Because CcrZ had an affinity to the resin even without the cysteine protease domain, instead of on-column tag cleavage, elution was collected with buffer containing 150 mM imidazole, 100 mM NaCl, 20 mM Tris pH 7.5 and 5 mM β-mercaptoethanol, and tag cleavage was performed for 1 h at 4 °C by adding 1 mM inositol hexakisphosphate. The sample was further purified using a HitrapQ column and Superdex 200 16/600 pg column (GE Healthcare). The final storage buffer contained 100 mM NaCl, 20 mM Tris pH 7.5 and 1 mM dithiothreitol. For antibody production, sample was loaded onto a 15% SDS–PAGE gel. Edge wells were cut out and stained with Coomassie to determine the position of CcrZ on the gel. Gel portions containing CcrZ were sent for antibody production by Eurogentec.

Western blot analysis

Cells were grown in C+Y medium until OD595 = 0.2 and harvested by centrifugation at 8,000g for 2 min at room temperature from 1 ml of culture. Cells were resuspended in 150 µl of Nuclei Lysis Solution (Promega) containing 0.05% SDS, 0.025% deoxycholate and 1% protease inhibitor cocktail (Sigma-Aldrich), and incubated at 37 °C for 20 min and at 80 °C for 5 min to lyse the cells. One volume of 4× SDS sample buffer (50 mM Tris–HCl pH 6.8, 2% SDS, 10% glycerol, 1% β-mercaptoethanol, 12.5 mM EDTA and 0.02% Bromophenol blue) was then added to three volumes of cell lysate sample and heated at 95 °C for 10 min. Protein samples were separated by SDS–PAGE (4–20%) and blotted onto polyvinylidene fluoride membranes (Merck Millipore). Membranes were blocked for 1 h with Tris-buffered saline (TBS) containing 0.1% Tween 20 (Sigma-Aldrich) and 5% dry milk and further incubated for 1 h with primary antibodies diluted in TBS, 0.1% Tween 20, 5% dry milk. Polyclonal CcrZ-antiserum concentration used was 1:5,000 and commercial polyclonal rabbit anti-GFP IgG (Invitrogen A-6455) was used at 1:5,000. Membranes were washed four times for 5 min in TBS, 0.1% Tween 20 and incubated for 1 h with secondary goat anti-rabbit IgG horseradish peroxidase-conjugated (Abcam AB205718) diluted 1:20,000 in TBS, 0.1% Tween 20 and 5% dry milk. Membranes were then washed four times for 5 min in TBS, 0.1% Tween 20 and revealed with Immobilon Western HRP Substrate (Merck Millipore).

CcrZ–GFP purification with anti-GFP nanobodies

gfp–ccrZ and P3–gfp (negative control) strains were grown in C+Y medium at 37 °C until OD595 = 0.2 and cells were harvested by centrifugation 15 min at 3,000g at 4 °C. Cells were then incubated in sucrose buffer (0.1 M Tris–HCl pH 7.5, 2 mM MgCl2, 1 M sucrose, 1% protease inhibitor cocktail (Sigma-Aldrich), 200 μg ml−1 RNase A and 10 μg ml−1 DNase (Sigma-Aldrich)) for 30 min at 30 °C, then incubated in hypotonic buffer (0.1 M Tris–HCl pH 7.5, 1 mM EDTA, 1% Triton, 1% protease inhibitor cocktail, 200 μg ml−1 RNase A and 10 μg ml−1 DNase) for 15 min at room temperature and cell debris were eliminated by centrifugation 30 min at 15,000g and 4 °C. Cell lysate was then incubated with equilibrated GFP-Trap resin (Chromotek) at 4 °C for 2 h. After several washes with wash buffer (10 mM Tris–HCl pH 7.5, 150 mM NaCl, 0.5 mM EDTA, 1% protease inhibitor cocktail), beads were resuspended in 20 µl of 8 M urea, 50 mM triethylammonium bicarbonate, pH 8.0 and reduced with 5 mM dithiothreitol for 30 min at 37 °C. Cysteines were alkylated by adding 20 mM iodoacetamide and incubated for 30 min at room temperature in the dark. Samples were diluted 1:1 with triethylammonium bicarbonate buffer, digested by adding 0.1 µg of modified trypsin (Promega) and incubated overnight at 37 °C, followed by a second digestion for 2 h with the same amount of enzyme. The supernatant was collected, diluted twice with 0.1% formic acid and desalted on strong cation-exchange micro-tips (StageTips, Thermo Fisher Scientific) as described previously60. Peptides were eluted with 1.0 M ammonium acetate (100 µl). Dried samples were resuspended in 25 µl of 0.1% formic acid, 2% acetonitrile prior being subjected to nano liquid chromatography tandem mass spectrometry (LC–MS/MS).

LC–MS/MS analysis

Tryptic peptide mixtures (5 µl) were injected on a Dionex RSLC 3000 nanoHPLC system interfaced via a nanospray source to a high-resolution QExactive Plus mass spectrometer (Thermo Fisher Scientific). Peptides were separated on an Easy Spray C18 PepMap nanocolumn (25 or 50 cm×75 µm ID, 2 µm, 100 Å, Dionex) using a 35 min gradient from 4 to 76% acetonitrile in 0.1% formic acid for peptide separation (total time: 65 min). Full mass spectrometry (MS) survey scans were performed at 70,000 resolution. In data-dependent acquisition controlled by Xcalibur v.4.0.27.19 software (Thermo Fisher), the ten most intense multiply charged precursor ions detected in the full MS survey scan were selected for higher energy collision-induced dissociation (normalized collision energy = 27%) and analysis in the orbitrap at 17,500 resolution. The window for precursor isolation was of 1.6 m/z units around the precursor and selected fragments were excluded for 60 s from further analysis.

MS data were analysed using Mascot v.2.5 (Matrix Science) set up to search the UniProt (www.uniprot.org) protein sequence database restricted to S. pneumoniae D39/NCTC 7466 taxonomy (339 SWISSPROT sequences + 1,586 TrEMBL sequences). Trypsin (cleavage at K,R) was used as the enzyme definition, allowing two missed cleavages. Mascot was searched with a parent ion tolerance of 10 ppm and a fragment ion mass tolerance of 0.02 Da (QExactive Plus). Iodoacetamide derivative of cysteine was specified in Mascot as a fixed modification. N-terminal acetylation of protein, oxidation of methionine and phosphorylation of Ser, Thr, Tyr and His were specified as variable modifications. Scaffold software (v.4.4, Proteome Software) was used to validate MS/MS-based peptide and protein identifications, and to perform data set alignment. Peptide identifications were accepted if they could be established at >90.0% probability as specified by the Peptide Prophet algorithm61 with Scaffold delta-mass correction. Protein identifications were accepted if they could be established at >95.0% probability and contained at least two identified peptides. Protein probabilities were assigned by the Protein Prophet algorithm62. Proteins that contained similar peptides and could not be differentiated based on MS/MS analysis alone were grouped to satisfy the principles of parsimony. Proteins sharing significant peptide evidence were grouped into clusters.

Split-luciferase assay

S. pneumoniae cells were grown in C+Y medium at 37 °C until OD595 = 0.2 and washed once with fresh C+Y medium. 1% NanoGlo Live Cell substrate (Promega) was then added, and luminescence was measured 15 times at 37 °C every 30 s in a plate reader (TECAN Infinite F200 Pro). Measurements were performed in triplicate and the average values were plotted, with the s.e.m. represented by the dot size.

Bacterial two-hybrid assay

The bacterial two-hybrid assay was based on the method from Karimova et al.32 with the following modifications. dnaA, ccrZ and ftsZ genes from S. pneumoniae D39V were cloned both into the low copy-number vector pUT18 and into the high copy-number vector pST2563 using the enzymes BamHI and KpnI. E. coli strain HM1784 (BTH101 Δrnh::kan) was transformed using each combination of plasmids. Chemically competent cells were incubated on ice for 60 min, heat shocking at 42 °C for 90 s and then inoculated at 37 °C in 3 ml of LB media supplemented with ampicillin (100 µg ml−1) and spectinomycin (50 µg ml−1) with mild agitation for 16 h. The OD600 was adjusted to 0.5, cultures were diluted 1:1,000 and a 5-µl aliquot was spotted on a nutrient agar plate containing antibiotics (as above) containing 0.006% X-gal. Plates were incubated at 30 °C for 48 h and the images were captured using a digital camera.

Co-immunoprecipitation of CcrZ and FtsZ–GFP with anti-GFP nanobodies

S. pneumoniae cells were grown in C+Y medium at 37 °C until OD595 = 0.2 and harvested by centrifugation 15 min at 3,000g at 4 °C. Cells were lysed using GFP–Trap_A Lysis buffer (Chromotek), 0.25% deoxycolate, 1% protease inhibitor cocktail incubated at room temperature for 10 min followed by incubation at 4 °C for 20 min. Cell lysate was incubated with equilibrated GFP-Trap resin (Chromotek) at 4 °C for 2 h. The resin was then washed three times in GFP-Trap_A Wash buffer (Chromotek) and GFP–proteins were eluted using SDS sample buffer at 95 °C for 10 min and analysed by immunoblotting.

Genome resequencing of ccrZ suppressors by next-generation sequencing

Strains hlpA–mKate2 ΔccrZ, ccrZsupp1, ccrZsupp2 and ccrZsupp3 were grown in C+Y medium at 37 °C until OD595 = 0.3 and cells were harvested by centrifugation for 1 min at 10,000g. Pellet was then resuspended into Nuclei Lysis Solution (Promega) containing 0.05% SDS, 0.025% deoxycholate and 200 µg ml−1 RNase A at 37 °C for 20 min to lyse the cells and Protein Precipitation Solution (Promega) was added. DNA was then precipitated using isopropanol. The extracted genomes were then analysed by Illumina sequencing by GATC Biotech (Eurofins Genomics). Mutations were mapped onto D39V genome using breseq pipeline64. Genomes sequences are available at SRA (project PRJNA564501).

oriC/ter ratios determination by RT–qPCR

Determination of S. pneumoniae oriC/ter ratios was performed as follows. Cells were pregrown until OD600 = 0.4 in C+Y medium at 37 °C, with or without inducer (ZnCl2 or IPTG) for complementation and depletion conditions, respectively. Cells were then diluted 100 times in fresh C+Y medium supplemented when appropriate with inducer and harvested for genomic DNA isolation when they reached OD600 = 0.1 (exponential phase). For normalization (oriC/ter ratio of 1), dnaA thermosensitive strain was grown for 2 h at non-permissive temperature (40 °C) in C+Y medium and harvested for chromosomal DNA isolation. As a negative (overinitiating) control, wild-type S. pneumoniae was incubated 2 h with 0.15 μg ml−1 HPUra (DNA replication inhibitor) at 37 °C before harvesting. Primers pairs OT1/OT2 and OT3/OT4 were used to amplify the oriC and ter regions, respectively. Amplification by RT–qPCR was performed in triplicate using SYBR Select Master Mix (Applied Biosystems) on a StepOne Plus Real-Time PCR System (Applied Biosystems). For S. aureus oriC/ter ratio determination, overnight cultures were diluted 100-fold and grown until OD600 = 0,4. These cultures were then re-diluted 200-fold in medium with 500 µM IPTG and grown until OD600 = 0.2. As reference samples with an assumed oriC/ter ratio of 1, wild-type S. aureus SH1000 cells at OD600 = 0.15 were supplemented with 50 µg ml−1 rifampicin (inhibiting replication initiation) and incubated for 2 h for replication run-out. Cells were then harvested and lysed enzymatically by addition of 0.2 mg ml−1 lysostaphin and 10 mg ml−1 lysozyme, and genomic DNA was isolated using the Wizard Genomic DNA Purification Kit (Promega). Quantitative PCR (qPCR) reactions of 10 µl were set up with 5 µl of PowerUpTM SYBR Green Master Mix (Applied Biosystems), 500 nM of each primer OT5/OT and OT7/OT8 and 20 ng of DNA. In both cases, amplification efficiencies of the primers and oriC/ter ratios were determined as described previously35. Data were plotted as a whisker plot in which whiskers represent the 25th and 75th percentiles of data from 10,000 Monte Carlo simulations, (*P < 0.05, values caluculated by bootstrap). For determination of B. subtilis oriC/ter ratios, cultures were grown to the mid-exponential phase in LB medium, diluted back to OD600 = 0.05 and grown to the mid-exponential phase (OD600 = 0.2–0.4) at 37 °C. Cells were harvested in ice-cold methanol (1:1 ratio) and pelleted. Genomic DNA was isolated using Qiagen DNeasy kit with 40 μg ml−1 lysozyme. The copy number of the origin (oriC) and terminus (ter) were quantified by qPCR to generate the oriC/ter ratio. qPCR was done using SSoAdvanced SYBR master mix and CFX96 Touch Real-Time PCR system (Bio-Rad). Primers used to quantify the origin region were OT9/OT10. Primers used to quantify the terminus region were OT11/OT12. Origin-to-terminus ratios were determined by dividing the number of copies (as indicated by the Cp values measured through qPCRs) of the origin by the number of copies quantified at the terminus. Ratios were normalized to the origin-to-terminus ratio of a temperature-sensitive mutant, dnaB134 (KPL69), that was grown to have synchronized replication initiation, resulting in a 1:1 ratio of the oriC/ter. Data were plotted as whisker plots where whiskers represent the 25th and 75th percentiles of data and the P value was obtained by a two-tailed t-test.

Genetic interactions determination by CRISPRi-seq

The protocol for CRISPRi library construction, sequencing and analysis was performed as described previously38. Briefly, 1,499 plasmids containing a different sgRNA were transformed into strain Ptet-dCas9, Plac-ccrZ, ∆ccrZ in the presence of 1 mM IPTG to ensure the expression of wild-type ccrZ, resulting in a pooled library containing the inducible CRISPRi system under control of an aTc-inducible promoter and combined with a depletion of ccrZ under control of an IPTG-inducible promoter. Colonies were harvested and stored at −80 °C. To ensure sufficient induction of the library, cells were grown for eight generations in triplicate. The pooled libraries were diluted 1:100 from stock in 10 ml of C+Y medium supplemented, or not, with 50 ng ml−1 aTc and 1 mM IPTG and grown at 37 °C. At OD600 = 0.4, cells were harvested and their genomic DNA isolated and prepared for MiniSeq (Illumina) sequencing with a custom sequencing protocol (www.veeninglab.com/crispri-seq). Significance of differential sgRNA depletion/enrichment between aTc treatments, across ccrZ complementation and depletion (absolute log2FC > 1, FDR-adjusted P < 0.05) was tested with the DESeq2 package as described previously38,65.

Capsule immunofluorescence

For fluorescence analysis of S. pneumoniae polysaccharide capsule, cells were grown in C+Y medium at 37 °C until OD595 = 0.1 and 1:1,000 diluted serum anti-serotype 2 from rabbit (Neufeld antisera, Statens Serum Institut 16745) was added for 5 min at 4 °C. Cells were washed three times with fresh C+Y medium and 1 mg ml−1 of superclonal recombinant secondary antibody goat anti-rabbit IgG coupled to Alexa Fluor 555 (Invitrogen A27039) was added for 5 min at 4 °C. Cells were then spotted onto a PBS–agarose slide. Acquisition of the fluorescent signal was performed on DV Elite microscope with mCherry filter set (Ex: 575/25 nm, BS: 605/50, Em: 632/60 nm).

Conservation and gene neighbourhood

The CcrZ protein sequence was aligned against all non-redundant protein sequences from NIH (ncbi.nlm.nih.gov) using PSI-BLAST for different Firmicutes families. Sequences with the highest identity were then aligned using Clustal Omega (ebi.ac.uk/Tools/msa/clustalo) and a phylogenetic tree was generated using Interactive Tree Of Life (itol.embl.de). Gene neighbourhood data were obtained from the STRING database (string-db.org). For residue conservation data, 1,000 sequences of CcrZ homologues were retrieved with PSI-BLAST (ebi.ac.uk) from the UniRef50 database. Conservation visualization was obtained using WebLogo 3 (weblogo.threeplusone.com). Sequences were then aligned using Clustal Omega and CcrZ sequence with conservation scores was mapped using UCSF Chimera (cgl.ucsf.edu/chimera) onto the crystal structure of S. pneumoniae LicA (PDB 4R78), the closest homologue protein using HMM–HMM comparison with HHpred20.

Statistics and reproducibility

Data analysis was performed using R (v.3.6.1). When comparing wild-type phenotypes with ccrZ depletion/complementation, a two-sided Wilcoxon rank sum test was used because we did not assume a normal distribution; some mutant cells can behave like wild-type because of the variable time of depletion or possible leakiness of Plac or PZn. When using box and whisker plots, the lower and upper quartiles, respectively, represent the 25th and 75th percentiles, the lower and upper whiskers represent, respectively, the 25th percentile + 1.5× interquartile range (IQR) and the 75th percentile + 1.5 IQR; the median is represented as a solid line. When plotting the oriC/ter ratios in Fig. 4, the outliers are also depicted by grey dots.

Data shown are represented as mean of at least three replicates ± s.e.m. if data came from one experiment with replicated measurement, and ± s.d. if data came from separate experiments. In general, each experiment shown in this paper was repeated independently at least two times with similar outcomes; n refers to the number of independent samples analysed per condition.

Reporting Summary

Further information on research design is available in the Nature Research Reporting Summary linked to this article.

Data availability

The data that support the findings of this study are available from the corresponding author on request. Data gathered from string-db are available at https://string-db.org. Published crystal structure of LicA in complex with AMP is available at PDB 4R78. SPD_0476 (CcrZ) amino acid sequence can be found in the UniProt Knowledgebase (uniprot/A0A0H2ZQL5). Genomes sequences data are available at NCBI Sequence Read Archive (SRA) under the following accession number PRJNA564501 and CRISPRi-seq data are available under accession number PRJNA740244. Source data are provided with this paper.

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Acknowledgements

We appreciate the assistance from the Electron Microscopy Facility (EMF) and the Protein Analysis Facility (PAF) at the University of Lausanne (UNIL) and thank them for their support. We thank Wiep Klaas Smits (LUMC) for the Split-luc sequences and Tanneke den Blaauwen (UVA) for the mTQox sequence before publication, Arnau Domenech (UNIL) for construction of strain hlpA–LgBit hlpA–SmBit and Zhian Salehian (NMBU) for help with cloning. Work in the Kjos laboratory is supported by a FRIMEDBIO grant (project number 250976) and a JPIAMR grant (project number 296906) from the Research Council of Norway. Work in the Murray laboratory was supported by a Wellcome Trust Senior Research Fellowship (204985/Z/16/Z) and a grant from the Biotechnology and Biological Sciences Research Council (BB/P018432/1). Work in the Grossman laboratory was supported, in part, by the National Institute of General Medical Sciences of the National Institutes of Health under award numbers R37 GM041934 and R35 GM122538. Work in the Veening laboratory is supported by the Swiss National Science Foundation (project grant 31003A_172861; NCCR ‘AntiResist’ 51NF40_180541; JPIAMR 40AR40_185533), a Novartis Foundation grant (#17B064) and ERC consolidator grant 771534-PneumoCaTChER.

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C.G. and J.-W.V. wrote the paper with input from all authors. C.G., S.S., M.E.A., Y.M.S., X.L., G.A.S., S.P., R.v.R., J.D. and M.K. performed the experiments. C.G., S.S., M.E.A., M.K., H.M., S.G., A.D.G. and J.-W.V designed, analysed and interpreted the data.

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Correspondence to Jan-Willem Veening.

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Peer review information Nature Microbiology thanks Joe Lutkenhaus, William Margolin and Hisao Masai for their contribution to the peer review of this work. Peer reviewer reports are available.

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Extended data

Extended Data Fig. 1 ccrZ deletion phenotype is conserved in S. aureus.

a, Left: CcrZ conservation in firmicutes. Percentages indicate the highest percent identity, for each class, obtained using PSI-BLAST with NIH sequences. Right: genes co-occurrence in several genomes (data obtained from string-db.org; see Methods). Horizontal section indicate complexity in neighborhood score assignment; white triangles indicate missing annotation. b, Growth curves at 37 °C and 30 °C of ccrZ depletion mutants using Plac (left) or PZn (right). c, Western blots for different pneumococcal strains. C: native CcrZ size; X: unknown protein recognized by α-ccrZ IgG. d, Microscopy of DAPI-stained S. aureus upon ccrZ silencing shows anucleate cells, while B. subtilis ΔccrZ mutant did not present nucleoid defects. Top and bottom scale bars, 3 µm; middle scale bar, 5 µm. ΔccrZ Sa cells were longer (or less well separated) and thinner (top right; wild type: n = 483 cells, ∆ccrZBs n = 399 cells; data are shown as box (25th to 75th percentile) and whiskers (1.5× IQR) plots with individual data points overlaid as dot plots) ***: P value = 6 × 10−29 and P value = 2 × 10−23 when comparing widths and lengths respectively, values derived from two-sided Wilcoxon rank sum test. Bottom-left: chromosome defects upon ccrZSa silencing can be rescued by expression of ccrZBs (ccrZSasgRNA-PccrZSa-ccrZBs + IPTG). Associated growth curves (bottom-right) also confirmed the complementation of ccrZSa by ccrZBs. e, Immunostaining of the polysaccharide capsule of S. pneumoniae wild type and upon ccrZ depletion. Scale bar, 3 µm.

Source data

Extended Data Fig. 2 Septal localization of CcrZ in S. pneumoniae.

a, Immunostaining of CcrZ in wild type S. pneumoniae shows a septal localization. Scale bar, 3 µm. b, Localization of CcrZ in other pneumococcal strains (un-encapsulated R6 strain and capsular serotype 4 TIGR4) and in S. aureus SH1000, as well as in B. subtilis 1A700. Left and top-right scale bars, 3 µm; bottom-right scale bar, 5 µm. c, 3D-SIM of GFP-CcrZ (green) and FtsZ-mCherry (red) and reconstructed volume projection of both. Left scale bar, 2 µm; right scale bar, 500 nm.

Extended Data Fig. 3 CcrZ controls DNA integrity.

a, Localization of the nucleoid associated protein HlpA in a ccrZ mutant shows anucleate cells. Scale bar, 3 µm. b, Mapping of DnaA Q247 and S292 residues onto the crystal structure of DnaA’s AAA+ and duplex-DNA-binding domains from Aquifex aeolicus. Both residues are predicted to be in the AAA+ domain. DnaA Q247 and S292 correspond to A. aeolicus DnaA Q208 and E252 respectively.

Extended Data Fig. 4 CcrZ activity is crucial for proper replication initiation as a dnaATS mutant phenocopied a ccrZ deletion.

a, Microscopy of DAPI-stained DnaA thermosensitive strain at non-permissive temperature (40 °C) indicates several anucleate cells, compared to a wild type grown in identical conditions. Scale bar, 3 µm. b, No interaction was detected between DnaA and CcrZ using bacterial-2-hybrid, while a positive DnaA-DnaA self-interaction is visible. c, Using split-luc assay, no interaction between CcrZ-YabA was detected, while a strong signal was obtained for DnaA-YabA. DnaA level was controlled by Plac to avoid toxicity. Each circle represents the average of n = 15 measurements of a technical replicate, with the size of the dot representing the SEM. d, Five (H157, D159, N164, D177 and D189) most conserved residues between 1,000 different CcrZ sequences from different bacterial species; sequences obtained from UniRef50 database.

Source data

Extended Data Fig. 5 Transient co-localization of CcrZ and DnaA.

Co-localization of CcrZ-mKate2 with DnaA-GFP (left) and corresponding heatmap of signal distribution over cell length (right) show that DnaA and CcrZ co-localize at the beginning of the cell cycle. Scale bar, 3 µm.

Supplementary information

Supplementary Information

Legends to Supplementary Videos 1–8, Methods, Tables 1–4 and references.

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Supplementary Video 1

3D-SIM of GFP–CcrZ in wild-type cells.

Supplementary Video 2

Time-lapse microscopy of GFP–CcrZ in live cells.

Supplementary Video 3

Time-lapse analysis of GFP–CcrZ and FtsZ–mCherry in live cells.

Supplementary Video 4

3D-SIM of GFP–CcrZ and FtsZ–mCherry in wild-type cells.

Supplementary Video 5

Time-lapse microscopy of CcrZ–mKate2 in FtsZ depleted cells.

Supplementary Video 6

Time-lapse analysis of HlpA–mKate2 in ΔccrZ cells.

Supplementary Video 7

Time-lapse microscopy of FtsZ–mTurquoise2 in DnaATS following temperature shift.

Supplementary Video 8

Time-lapse analysis of CcrZ–mKate2, DnaN–sfTQOX and ParBp–sfmYFP in live cells.

Source data

Source Data Fig. 1

Numerical source data for Fig. 1g.

Source Data Fig. 2

Numerical source data for Fig. 2e.

Source Data Fig. 3

Numerical source data for Fig. 3a.

Source Data Fig. 3

Unprocessed membranes and gel images for Fig. 3c,d.

Source Data Fig. 4

Numerical source data for Fig. 4f–j,l,n,o.

Source Data Fig. 5

Numerical source data for Fig. 5c.

Source Data Fig. 6

Numerical source data for Fig. 6d.

Source Data Extended Data Fig. 1

Numerical source data for Extended Data Fig. 1d.

Source Data Extended Data Fig. 1

Unprocessed membranes images for Extended Data Fig. 1c.

Source Data Extended Data Fig. 4

Numerical source data for Extended Data Fig. 4c.

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Gallay, C., Sanselicio, S., Anderson, M.E. et al. CcrZ is a pneumococcal spatiotemporal cell cycle regulator that interacts with FtsZ and controls DNA replication by modulating the activity of DnaA. Nat Microbiol 6, 1175–1187 (2021). https://doi.org/10.1038/s41564-021-00949-1

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