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Journal of Bacteriology, September 2006, p. 6629-6639, Vol. 188, No. 18
0021-9193/06/$08.00+0     doi:10.1128/JB.00672-06
Copyright © 2006, American Society for Microbiology. All Rights Reserved.

Sequence Analysis of the Lactococcal Plasmid pNP40: a Mobile Replicon for Coping with Environmental Hazards{dagger}

Jonathan O'Driscoll,1 Frances Glynn,1 Gerald F. Fitzgerald,1,2 and Douwe van Sinderen1,2*

Department of Microbiology,1 Alimentary Pharmabiotic Centre, University College Cork, Cork, Ireland2

Received 11 May 2006/ Accepted 28 June 2006


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ABSTRACT
 
The conjugative lactococcal plasmid pNP40, identified in Lactococcus lactis subsp. diacetylactis DRC3, possesses a potent complement of bacteriophage resistance systems, which has stimulated its application as a fitness-improving, food-grade genetic element for industrial starter cultures. The complete sequence of this plasmid allowed the mapping of previously known functions including replication, conjugation, bacteriocin resistance, heavy metal tolerance, and bacteriophage resistance. In addition, functions for cold shock adaptation and DNA damage repair were identified, further confirming pNP40's contribution to environmental stress protection. A plasmid cointegration event appears to have been part of the evolution of pNP40, resulting in a "stockpiling" of bacteriophage resistance systems.


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INTRODUCTION
 
Lactococcus lactis, a gram-positive lactic acid bacterium, has been extensively exploited for the production of a variety of fermented dairy products. L. lactis strains exhibit biotechnologically important activities, which contribute to the character of the final food product, e.g., lactose utilization and protease production, and in addition encode properties that specifically provide a selective advantage to the bacterium itself, e.g., heavy metal resistance, bacteriocin production and/or immunity, and bacteriophage resistance (47). Many of these industrially significant traits have been found to be encoded by plasmids, which are omnipresent among this species, with most isolates containing multiple plasmids ranging in size from 2 to 80 kb (11).

In recent decades, extensive research has established the molecular mechanisms governing many of these activities, in particular with respect to bacteriophage resistance (47). Lactococcal strains used for many food fermentations are known to be persistently challenged by phages and probably as a consequence have evolved numerous bacteriophage resistance strategies (48, 67).

Presently, there are 30 completely sequenced lactococcal plasmids, the largest being pSK11P, a 75.8-kb plasmid isolated from L. lactis subsp. cremoris SK11 (47, 62). This plasmid encodes a variety of functions, including copper resistance, proteolytic activity, cold shock proteins, and cation transport activities, and displays clear "markings" of multiple recombination events that may have contributed to its evolution (62).

Previous studies of a similarly sized plasmid, pNP40, originally identified in L. lactis subsp. diacetylactis DRC3 (45), revealed that this molecule, besides its encoded nisin and cadmium resistance determinants, is responsible for an impressive bacteriophage resistance profile (16, 19, 20, 50, 65). Two such systems, AbiE and AbiF, were found to provide significant resistance that correlates to an abortive infection phenotype (19).

In addition, on the basis of phenotypic evidence, the presence of a third mechanism active at the stage of phage DNA injection was proposed (20). Most recently, a fourth resistance system, the LlaJI restriction-modification system, was identified (50).

In the present study, we report the complete sequence of pNP40. Analysis of the sequence revealed the genetic determinants involved in replication and conjugation, in addition to genes responsible for previously uncharacterized functions. Furthermore, evidence is offered which attests to pNP40's full bacteriophage resistance potential.


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MATERIALS AND METHODS
 
Bacteria, bacteriophage, plasmids, media and growth conditions. Details of the bacterial strains, bacteriophages, and plasmids used in the present study are summarized in Table 1. All L. lactis strains were grown in M17 broth (Oxoid ltd., Hampshire, United Kingdom) containing 0.5% glucose at 30°C. Escherichia coli was grown at 37°C in Luria-Bertani (LB) medium (58). Where appropriate, antibiotics were added as follows: for L. lactis, tetracycline at 5 µg ml–1, chloramphenicol at 10 µg ml–1, and erythromycin at 1 µg ml–1; for E. coli, ampicillin at 100 µg ml–1, kanamycin at 25 µg of ml–1, chloramphenicol at 10 µg ml–1, and erythromycin at 100 µg ml–1. LB medium was supplemented with X-Gal (5-bromo-4-chloro-3-indolyl-ß-D-galactopyranoside; 40 µg ml–1) and IPTG (isopropyl-ß-D-thiogalactopyranoside; 1 mM) where appropriate. Recombinant L. lactis cells containing pAK80 and derivatives were selected on GM17 agar (containing 0.5 M sucrose) with erythromycin, supplemented with X-Gal (40 µg ml–1). Lactococcal bacteriophage were propagated as described previously (50). Plaque assays were conducted as described elsewhere (41) and the efficiency of plaquing (EOP) was calculated as the ratio of the number of plaques formed on a tested host to those formed on a sensitive host.


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  		TABLE 1. Bacteria, bacteriophages, and plasmids used in this study

Molecular techniques and shotgun cloning. Restriction enzymes and T4 DNA ligase were purchased from New England Biolabs (Hertfordshire, United Kingdom) and used according to the manufacturer's instructions. E. coli plasmid DNA was isolated by using the SV Wizard plasmid miniprep kit (Promega, Madison, WI). Routine lactococcal plasmid DNA isolations were performed as described previously (52). Isolation of pNP40 plasmid DNA for shotgun cloning was performed as described previously (2), and the resulting DNA preparation was purified by cesium chloride-ethidium bromide density gradient ultracentrifugation using standard techniques (58). Electroporation of plasmid DNA into E. coli was performed by using standard techniques (58) and in L. lactis as described previously (69). Purified pNP40 DNA was digested with HindIII, EcoRI, and XbaI separately and shotgun cloned into the E. coli plasmid pBluescript KS(–). Large restriction fragments (>5 kb) were further digested with DraI, Sau3A, or HaeII prior to cloning in pBluescript. For routine PCR applications Taq DNA polymerase (QIAGEN, West Sussex, United Kingdom) was used. For plasmid construction, where high fidelity was required, PCRs were conducted by using a combination of Taq DNA polymerase and Proofstart DNA polymerase (QIAGEN) according to the manufacturer's instructions. All PCR products were purified by using the Jetquick PCR purification kit (Genomed, Lohne, Germany). The correct orientation and integrity of all constructs was verified by sequencing, performed at MWG Biotech (Ebersberg, Germany).

Sequence assembly and annotation. Sequence assembly, verification, and analysis of pNP40 and plasmid constructs were achieved by using the SeqMan program from the DNASTAR package (DNASTAR, Madison, WI). Initial annotation was performed automatically using the open reading frame (ORF) finder tool from the National Center for Biotechnology information (http://www.ncbi.nlm.nih.gov/) and the DNASTAR software package. Potential ORFs were subsequently manually analyzed by database searches using the BLAST suite of programs (including blastp, clusters of orthologous groups [COG], conserved domain database [CDD], and the conserved domain architecture tool [CDART]) (1), which incorporate domains imported from the simple modular architecture research tool (SMART) (40) and the protein family database (Pfam) (15). Additional searches were performed by using the CBS prediction servers (http://www.cbs.dtu.dk/services/). The complete nucleotide sequence of pNP40 has been deposited in the GenBank database under accession no. DQ534432.

Plasmid constructs. All of the oligonucleotide sequences (and coordinates) used for plasmid construction are available online (see Table S2 in the supplemental material). For the construction of plasmid pAKC, a PCR product encompassing the assumed cspC promoter region (using primers AKCF and AKCR) was inserted into the HindIII-BglII sites of pAK80. For pAKD, a PCR product encompassing the assumed cspD promoter region (using primers AKDF and AKDR) was inserted into the HindIII-BglII sites of pAK80. For pNZ-CD, a cspCD-encompassing PCR product which also included both cspC and cspD promoter regions (using primers cspCF and cspDR) was inserted into the NcoI-PstI sites of pNZ8048. Plasmid pAK17 was constructed by insertion of a PCR product encompassing the orf17 upstream region (using primers orf17F and orf17R) into the HindIII-BglII sites of pAK80. For pAK18, a PCR product encompassing the upstream orf18 region (using primers orf18F and orf18R) was inserted into the HindIII-BglII sites of pAK80. For pAK25, a PCR product encompassing the upstream region of orf25 (using primers orf25F and orf25R) was inserted into the HindIII-BglII sites of pAK80. Plasmid pORF1 was constructed by insertion of a PCR product encompassing orf1 and its presumed transcriptional signals (using primers orf1F and orf1R) into the BglII site of pPTPi. Plasmid pORF13 was constructed by insertion of an orf13 encompassing PCR product (using primers orf13F and orf13R) into the NcoI-Asp718 sites of pNZ44. Plasmid pNZ-6.2 was constructed by insertion of a 6.2-kb NcoI fragment of pNP40 (coordinates 21824 to 28061) into the NcoI site of pNZ8048. For plasmid pNZ-7, a 7-kb NcoI fragment of pNP40 (coordinates 14786 to 21823) was inserted into the NcoI site of pNZ8048. Plasmid pNZ-10 was constructed by insertion of a 10-kb NcoI fragment of pNP40 (coordinates 32175 to 42226) into the NcoI site of pNZ8048.

Intracellular phage DNA replication. Lactococcal strains were grown to the early logarithmic growth phase (optical density at 600 nm [OD600] of ~0.3), after which CaCl2 was added to a final concentration of 10 mM, and the cells were infected with the {phi}sk1 or {phi}sk1.m (as indicated) at a multiplicity of infection of 0.1. Intracellular phage DNA replication was monitored as described previously (28). DNA preparations were separated by electrophoresis on a 1% agarose gel and transferred to a Hybond-N+ nylon membrane (Amersham, United Kingdom) by capillary transfer using 10 mM NaOH. Membranes were probed with a {phi}sk1-specific PCR product (generated by using the primers SK1F [5'-GGCTATATGCTCATATTTTGG-'3] and SK1R [5'-CTCTCACCGCCATATTGTC-'3]) using the ECL direct nucleic acid labeling and detection system (Amersham) according to the manufacturer's instructions. Control phage DNA was isolated from lysates as described previously (49).

Freeze-thaw challenge and DNA damage assays. Freeze-thaw challenge experiments were performed essentially as described elsewhere (71, 72). Briefly, cells were grown in GM17 medium at 30°C to an OD600 of 0.5 and subjected to a cold shock by rapid temperature downshift from 30 to 10°C for 0, 2, or 4 h, after which 1 ml of these cultures was frozen at –20°C. After a 24-h freezing period, the cells were allowed to thaw at 30°C for 4 min with subsequent survival of strains assayed by determining viable counts. This freeze-thaw cycle was performed four times. Sensitivity to chemically induced DNA damage was assayed by inclusion of mitomycin C (MMC; 2.5 µg ml–1) in growth media. Cells were grown to early log phase (OD600 ~0.2), at which point the mutagen was added, followed by monitoring of growth by means of OD600 measurement. Viable counts were performed at selected time points to corroborate OD600 measurements.

ß-Galactosidase assays. ß-Galactosidase assays were performed essentially as described previously (30). For analysis of cold shock-induced transcription, cells containing various lacZ-transcriptional fusions were grown to an OD600 of 0.5 and subjected to a cold shock at 10°C for 0, 2, and 4 h, after which 1-ml samples were harvested and analyzed for ß-galactosidase activity.

For analysis of DNA damage-induced gene expression, cells containing various lacZ transcriptional fusions were grown to OD600 of 0.2 to 0.3, followed by the addition of MMC (2.5 µg ml–1), after which 1-ml samples were harvested at 0, 15, 30, 60, and 90 min and analyzed for ß-galactosidase activity.

Construction of a pNP40 deletion derivative. The deletion derivative of pNP40 was constructed by targeted deletion mutagenesis as described previously (10, 37, 38). Briefly, two PCR products, A and B, flanking the region of pNP40 to be deleted, were generated. Product A was amplified by using primers M1Fa and M1Rb, whereas product B was amplified by using primers M1Fc and M1Rd, and the two resulting DNA fragments were joined by SOEing PCR as described previously (29). This SOEing product was then inserted into the NcoI-BamHI sites of the integration vector pOri280 (RepA–) in the E. coli cloning host EC101 (RepA+), to generate plasmid pSoe1. Plasmid pSoe1 was subsequently established in the MG1614/pNP40 background and selected for first and second crossover events. The integrity of the pNP40 deletion derivative, pNP40{Delta}Soe1, was verified by PCR, Southern hybridization, and sequencing.


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RESULTS AND DISCUSSION
 
Plasmid sequence and genetic organization. The conjugative lactococcal plasmid pNP40, originally identified in L. lactis subsp. diacetylactis DRC3 (45), was established in the plasmid-free lactococcal strain MG1614, from which plasmid DNA was subsequently purified and sequenced (as outlined in the Materials and Methods). Assembly of the resulting sequences resulted in a single contiguous contig representative of a circular 64,980-bp DNA molecule with a G+C content of 32.33%. This is somewhat lower than that of L. lactis chromosomal DNA (35.4% for IL1403 [4], 35.8% for MG1363 [34], and 35% for SK11 [Joint Genome Institute]) but is within the range exhibited by most sequenced lactococcal plasmids to date (30 to 40%) (47). A total of 62 ORFs were identified in the pNP40 sequence, which were analyzed in detail below (see Materials and Methods, Fig. 1, and Table S1 in the supplemental material).


Figure 1
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  		FIG. 1. Genetic map of the lactococcal plasmid pNP40. Block arrows and lines represent identified ORFs. A number of functional gene clusters are indicated.

pNP40 replication functions. Previous work had localized the minimal replicon for pNP40 to a cloned 7.6-kb EcoRI fragment, which also expressed a nisin resistance activity (see below) (16). Further subcloning suggested that the replication functions were localized on a 5.0-kb EcoRI-XbaI fragment, corresponding to coordinates 59625 to 64637 of the pNP40 sequence. This region was found to contain orf59 (designated repA), orf60 (designated repB), and orf61 (see Table S1 in the supplemental material and Fig. 2A).


Figure 2
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  		FIG. 2. (A) Genetic organization of the replication region of pNP40. B. Sequence of repA and upstream and downstream regions. Translational start sites of repA and repB are in boldface, presumed ribosome-binding sites are underlined, and predicted consensus –10 and –35 sequences of the repB promoter are shaded. Inverted repeat structures are represented by opposing arrows, and the 40-bp directly repeated putative iteron sequences are indicated by the dashed arrows.

Analysis of the amino acid sequence of RepA revealed similarity to a number of pLS32-type theta replication proteins, including that of pCI2000 (AAF27326) from Lactococcus (73% identity). Consistent with this was the presence of a replication initiation N-terminal domain (pfam06970), which was noted to contain a helix-turn-helix motif (amino acid [aa] 68 to 89). Analysis of the coding region of RepA revealed the presence of a 40-bp sequence directly repeated two and three quarter times (Fig. 2B; additional features are as indicated). Such repeats, also termed iterons, are common elements of the origin of replication (ori) for many theta replicating plasmids (12, 25, 33, 35). Interestingly, the pLS32 ori is believed to be similarly located within the coding sequence for its replication initiation protein, RepN (63). This intragenic iteron locality was also noted for the pNP40 RepA homologue present on pCI2000 (31).

Located upstream of repA and transcribed divergently, repB is predicted to encode a gene product, which exhibits significant similarity to a number of replication-associated proteins from gram-positive plasmids (see Table S1 in the supplemental material), while containing SoJ (COG1192), Mrp (COG0489), and COG0455 domains, thus making it a member of the ParA ATPase family (pfam00991) involved in plasmid and chromosome partitioning. An equivalent ParA-type protein has previously been associated with an active plasmid partitioning system, and RepB likely mediates an equivalent stability function (31).

Immediately downstream of repB, a small coding region, orf61 is present. Homologous RepB-linked coding regions have been noted in many theta replicons which, due to their proximity and apparent transcriptional and/or translational coupling to RepB, are thought to be involved in the replication-partitioning process (3, 5, 25).

The genetic organization, similarities, and iteron structure of the pNP40 replication region strongly suggests that this large plasmid replicates via a theta-type mechanism. Furthermore, and typical of theta replicating plasmids, pNP40 appears to contain determinants that contribute to its high segregational stability (45).

Conjugal transfer determinants. In other microorganisms the structure and function of the conjugative apparatus has been examined in detail (18, 26, 36, 39). The conjugal capacity of pNP40 has previously been phenotypically demonstrated (27, 65). On the basis of similarity searches of the pNP40 sequence, we predict the presence of a conjugal transfer gene cluster on an approximately 17-kb section (coordinates 44565 to 61395), which contains 19 ORFs (orf40 to orf58) arranged in an operon structure (Fig. 3A and Table S1 in the supplemental material). The protein specified by orf58 (designated MobD) exhibits homology to the nickase-relaxase family of proteins (pfam03432), which introduce a nick at the origin of transfer (oriT) to initiate single-stranded plasmid DNA transmission from the donor to a recipient cell. A number of inverted repeat structures, reminiscent of an oriT, were identified downstream of the MobD coding region which was noted to be significantly AT-rich (~70%) (Fig. 3B). However, no obvious candidate consensus nick site (26) is present within this putative oriT.


Figure 3
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  		FIG. 3. (A) Genetic organization to the pNP40 conjugation region (Top). Checkered arrows represent ORFs encoding predicted membrane-spanning proteins. Conserved gene clusters (and percent identities) similar to segments of the conjugal transfer region of the enterococcal plasmids pCF10 and pAM373 are indicated. (B) Sequence of the region downstream of the mobD gene, predicted to contain the oriT. The mobD translational stop codon is in boldface, and the putative transcriptional terminator for the conjugation operon is indicated by opposing arrows (IR1). A perfect 22-bp inverted repeat (IR2) is indicated; this repeat was also noted to constitute two perfect 22-bp tandem repeats.

The pNP40 conjugation region appears to consist of modules each of which displaying sequence similarity to discrete sections from assumed conjugation regions from enterococcal plasmids (Fig. 3A). The notable exceptions include orf44, orf45, and orf53, which appear to represent components unique to pNP40. The product encoded by orf54 (designated TraF) is a membrane-spanning protein likely to be involved in mating channel formation, whereas ORF55 was noted to contain the "antirestriction" domain COG4227, in addition to a conserved H-E-X-X-K catalytic active site, and likely provides a temporal protection to the transferred plasmid DNA against restriction endonucleases, allowing establishment in the recipient cell (70).

The orf43 and orf48 gene products correspond to the conserved TraG (cd01126) (pfam02534) and TraE (COG3451) conjugation proteins, respectively, whose conserved domains are suggestive of a type IV secretion function (9, 23, 24, 61).

Both ORF49 and ORF50 exhibit homology to distinct regions within the protein product of ep0036 on pAM373 (AAG40447). ORF49 contains a conserved FlgJ muramidase domain (COG1705), whereas ORF50 contains a CHAP amidase domain (pfam05257), in contrast to EP0036, which contains both. These conserved domains are present in cell wall-metabolizing proteins; therefore, it can be speculated that ORF49 and ORF50 participate in facilitating the passage of DNA and/or proteins across the cell envelope by virtue of their peptidoglycan-degrading activity.

Cadmium resistance. Previously, the cadmium resistance encoded by pNP40 has been demonstrated to be a selectable marker for pNP40 dissemination to an industrial starter culture (65). Furthermore, the presence of a CadA homologue was confirmed by PCR using primers specific for the previously published CadA homologue of pAH82 (51).

The cadmium resistance region of pNP40 was found to reside in a section encompassed by coordinates 40808-43281, where two similarly oriented overlapping coding regions were distinguished (ORF36 and ORF37). The first ORF, ORF36, corresponds to the previously identified cadA homologue (65), whose product contained conserved domains consistent with proteins involved with Cu, Cd, Co, and Zn transport and detoxification (cdd00371), inorganic ion transport (COG2608), and cation transport (COG2217, pfam00122, pfam00702, COG0474, COG2216, and COG4087). The presence of these conserved regions indicates that the CadA activity spectrum is not solely restricted to cadmium efflux, as has previously been reported for other homologues (60).

The protein encoded by orf37 was found to be 100% identical to an abundance of CadC proteins, all of which were encoded by genes adjacent to CadA homologues. CadC was noted to possess a number of helix-turn-helix containing conserved domains (cdd00090, smart00418, and CAG0640) typical of homodimeric repressors, which dissociate from their target DNA in the presence of metal ions.

Nisin resistance region. As with cadmium resistance, the nisin resistance capabilities of pNP40 have been documented (16, 45). The sequenced nisin resistance gene, designated nisR, was located on a 1.8-kb EcoRI-KpnI fragment (coordinates 803 to 2584) (17). Analysis of the amino acid sequence of NisR confirmed the presence of an N-terminal membrane-spanning domain (aa 7 to 29) (but no signal peptide sequence) as suggested by Froseth and McKay (17) and further revealed the presence of conserved protease-peptidase domains (smart00245 and pfam03572) spanning approximately 200 aa at the C terminus, which was predicted to reside outside the cell membrane. From this it can be inferred that the mechanism of NisR-mediated nisin resistance occurs via proteolytic degradation of nisin.

Located immediately downstream and convergently oriented to the nisR gene, orf1 is predicted to encode an integral membrane protein containing a conserved, C-terminally located Abi, CAAX amino-terminal protease domain (pfam02517), which is typical of this diverse family of metal-dependent membrane proteases that are involved in protein and peptide modification and secretion (53). It has been suggested that these proteins may also play a role in bacteriocin maturation and transport and in resistance (14, 53).

Cold shock determinants. The protein products of two similarly oriented open reading frames, ORF38 and ORF39, are identical or nearly identical to the cold shock proteins CspD and CspC, respectively, of lactococcal chromosomal or plasmid origin. In addition, both conserved "cold shock" DNA- and RNA-binding domains (pfam00313 and smart00357, respectively) were observed within the pNP40-encoded CspC and CspD amino acid sequences.

Previous studies on the chromosomal CspC and CspD homologues have illustrated the physiological response mediated by these cold shock proteins; expression of CspD was enhanced by cold shock and resulted in increased survival at low temperatures, whereas only a modest increase in CspC expression accompanied cold shock, which was found to directly alter the levels of other cold shock proteins (71-73).

Transcriptional fusions of both the cspC and the cspD promoter regions of pNP40 showed that both promoters were induced by cold shock in a manner that was independent of the presence of pNP40 (Fig. 4A and B). The presence of these cold shock-related determinants on pNP40 suggests that this plasmid mediates an enhancement of the cold shock response. An analysis of the freeze-thaw survival capacity of MG1614 containing pNP40 compared to the plasmid-free strain illustrated a small but appreciable increase in survival (Fig. 4C), which was also observed with a construct containing the cspC and cspD genes cloned in tandem (pNZ-CD; data not shown).


Figure 4
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  		FIG.4. (A) ß-Galactosidase assays of the cspC promoter transcriptional fusion (present on pAKC) after 2 and 4 h of cold shock at 10°C. The graph depicts the fold increase in promoter activity after cold shock treatment relative to the promoter activity under non-cold-shock conditions (i.e., 30°C). Bars: 1, MG1614/pAKC (2 h at 10°C); 2, MG1614/pAKC (4 h at 10°C); 3, MG1614/pNP40/pAKC (2 h at 10°C); 4, MG1614/pNP40/pAKC (4 h at 10°C). Absolute values are listed beneath the graph. (B) ß-Galactosidase assays of the cspD promoter transcriptional fusion (present on pAKD) after 2 and 4 h of cold shock at 10°C. The graph depicts the fold increase in promoter activity after cold shock treatment relative to the promoter activity under non-cold-shock conditions (i.e., 30°C). Bars: 1, MG1614/pAKD (2 h at 10°C); 2, MG1614/pAKD (4 h at 10°C); 3, MG1614/pNP40/pAKD (2 h at 10°C); 4, MG1614/pNP40/pAKD (4 h at 10°C). Absolute values are listed beneath the graph. (C) Survival of MG1614 and MG1614/pNP40 frozen at –20°C after successive freeze-thaw cycles after exposure to a cold shock at 10°C for 0, 2, and 4 h as indicated.

The full phenotypic potential associated with these pNP40-encoded determinants, while clearly inducible, is likely only to be significantly detectable in a host (perhaps the original pNP40-containing host [45]) that does not encode chromosomal or plasmid cspC and cspD copies (or possibly under alternative stress or cold shock conditions).

DNA damage repair. pNP40 was found to possess three ORFs—ORF17, ORF18, and ORF25—which were predicted to encode proteins involved in DNA repair. The RecA (ORF18) and UmuC-like (ORF17) homologues, designated RecALP and OrfU, respectively, have been described previously (19, 21) (see Table S1 in the supplemental material and Fig. 1).

Analysis of the amino acid sequence of RecALP revealed the presence of multiple conserved domains characteristic of bacterial RecA homologues involved in homologous recombination, DNA repair, and SOS response induction (cd00983, cd01393, cd01120, and pfam00154). Adjacent and similarly oriented with respect to recALP, the orf17 gene encodes the UmuC-like protein, OrfU, which contains two conserved domains: the IMS (impB/mucB/samB) family (pfam00817; UV protection) and DinP (COG0389; DNA repair DNA polymerases). The UmuC family of proteins are an essential component of the DNA damage mutagenesis mechanism of E. coli and constitute the catalytic subunit of DNA polymerase V, which possesses a translesion DNA synthesis activity at the expense of normal replicative fidelity (54, 55, 64, 68).

The product of orf25 was predicted to harbor an UvrA exinuclease domain (COG0178) containing conserved, interrupted, N- and C-terminal ABC-ATPase motifs and similarly located zinc fingers. UvrA-type proteins are believed to comprise the ATPase subunit of the UvrABC nucleotide excision repair system (66). BLAST searches of the ORF25 (designated UvrA) amino acid sequence revealed 64% identity to UvrA of Lactobacillus plantarum WCFS1 (CAD63845) and 62% identity to UvrA of L. caseii ATCC 334 (ZP_00386320).

The presence of pNP40-encoded components of DNA repair systems prompted us to investigate the growth and survival of a pNP40-containing host in response to chemical-induced DNA damage. To this end, MG1614 containing pNP40 was challenged with MMC, and its growth profile was monitored. As can be seen from Fig. 5A, a significant difference in the growth profile was evident for the pNP40-containing host compared to that of the control strain in response to MMC. The pNP40-containing strain not only reached a higher final optical density but also did not lyse to the same extent as the control strain. The optical density values described were corroborated by viable plate counts (data not shown).


Figure 5
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  		FIG. 5. (A) Growth of MG1614 and MG1614/pNP40 in response to MMC. The arrow on the graph indicates when MMC was added to the culture. (B) ß-Galactosidase assay of the orfU promoter transcriptional fusion (pAK17) in the MG1614 host background at 15, 30, 60, and 90 min after exposure to MMC. The graph depicts the fold increase in promoter activity (and the P value) in the presence of MMC relative to the promoter activity at each time point in the absence of MMC. (C) Sequence of orfU, umuC (IL1403), and hdiR upstream regions. The –10 and –35 sequences are shaded, and the orfU start codon is in boface. Sequences corresponding to the core HdiR binding motif (ATCAGW5CTGAT) are underlined.

To establish whether the expression of orfU, recALP, and uvrA was induced in response to MMC, transcriptional fusions were constructed (see Materials and Methods). Of these, only the upstream regions of orfU and uvrA were found to contain active (but relatively weak) promoters (in the absence of MMC) in a lactococcal host. The upstream recALP region apparently did not contain any active transcriptional signals (in the presence or absence of MMC). Given that recALP-specific mRNA was detectable by dot blot analysis and the apparently identical recALP and orfU transcriptional yields (21), it is likely that these genes constitute a dicistronic operon transcribed from the orfU promoter. This may account for the inability of a cloned recALP to complement a chromosomal recA mutant (21), since recALP expression may not be entirely synchronized with that of the chromosomal version (see below).

As can be seen from Fig. 5B, expression from the orfU promoter was induced up to threefold when monitored for 90 min after exposure to MMC (which was not influenced by the presence of pNP40 [data not shown]), whereas no such increase in transcriptional activity was observed for the uvrA promoter. The latter promoter appears to be constitutive during exponential growth and increases in activity up to two- to threefold during early stationary phase in the absence of a DNA-damaging agent (data not shown). This lack of induction of uvrA in response to DNA damage, although in contrast to that observed for E. coli (32) and B. subtilis (8), is consistent with that noted for a uvrA homologue of Pseudomonas aeruginosa (56).

Analysis of the sequence of the inducible orfU promoter region revealed the presence of a conserved "HdiR" box (59) (Fig. 5C). HdiR is a LexA-like DNA damage regulator of L. lactis MG1363 and was shown to regulate the expression of the orfU homologue (umuC) from L. lactis IL1403 in addition to its own gene in response to MMC (59). Interestingly, MG1363 does not possess an umuC homologue (59). It is therefore likely that the observed induction of orfU from pNP40 in the presence of MMC is mediated by HdiR derepression. The uvrA promoter lacks "HdiR box"-resembling sequences, which is consistent with its expression pattern.

Insertion sequence elements: did pNP40 evolve as a result of cointegration? Insertion sequence (IS) elements are known to contribute significantly to species evolution (47, 57). Six IS elements were identified on the pNP40 sequence, only two of which (encoded by orf7 and orf35) appeared to be complete. Both ORF7 (227 aa) and ORF35 (194 aa) were found to be highly similar to ISS1 of the lactococcal plasmid pTD1 (CAA44601) and contained conserved integrase (pfam00665) and transposase (COG3316) domains. This almost exact ISS1 duplication on pNP40 suggests that the intervening region between orf7 and orf35 may have been acquired by an insertion event.

ISS1 is a member of the IS6 family, whose insertion sequences thus far have been noted to give rise exclusively to cointegrant replicon fusions (43). Downstream of the abiF gene within the ISS1-flanked section of pNP40, a 23-bp sequence repeated three and a half times (reminiscent of the iteron-containing origin of replication from some theta plasmids) has previously been reported (19). In addition, the orf8-to-orf10 region (in particular orf10) appear(s) to encode plasmid stability and maintenance determinants. The presence of these coding regions, and the iteron-like sequences mentioned above suggest that this section may have at some stage been capable of autonomous replication. These observations provide evidence which corroborates suggestions that pNP40 may have evolved as a result of a cointegration event (19).

The four remaining IS elements of pNP40 (orf23, orf24, orf26, and orf62) all encode apparent truncated and/or inactivated derivatives of members of the IS3 family (whose genetic organization usually consists of two genes translated together as a single polypeptide via translational slippage (6, 43).

The fourth bacteriophage-resistance phenotype: injection blocking versus synergy. Two abortive infection phage resistance systems (AbiE and AbiF) (19) and a putative DNA penetration blocking system (20) have been reported to reside on pNP40. Evidence for the latter system was initially based on the enhanced pNP40-mediated resistance to {phi}c2 compared to the level of resistance afforded by AbiF alone, with the observed phenotype noted to act prior to AbiF-mediated cell killing. The discovery of an active pNP40-encoded restriction-modification system, LlaJI (50) (which fulfills most of the penetration blocking phenotypes (20), made it essential to redefine the residual pNP40-mediated phage resistance activity. A small isometric-headed phage, {phi}sk1, was selected for this analysis since this phage could grow with apparently equal efficiency on a host containing either AbiE or AbiF alone. Although {phi}sk1 was restricted by a host containing the LlaJI system, propagation of surviving phage on the same LlaJI-containing host yielded completely LlaJI-insensitive progeny. These methylated phage ({phi}sk1.m) were therefore expected to be insensitive to all characterized phage resistance systems present on pNP40 and ideal for detection of any remaining unidentified resistance mechanism (provided {phi}sk1.m was sensitive to such a system).

As can be seen from Table 2, {phi}sk1.m formed plaques with equal efficiency on all strains (although slightly tighter plaques were formed on the AbiE-containing host), with the exception of the host possessing pNP40, confirming the presence of a residual resistance phenotype against this phage. In addition, accumulation of intracellular {phi}sk1.m DNA was considerably delayed in the pNP40-containing host compared to that of the sensitive host (Fig. 6). Here, a high intracellular {phi}sk1.m DNA concentration was detected in the control MG1614 host after 40 min, with lysis ensuing. In the pNP40-containing host, an equivalent concentration of intracellular {phi}sk1.m DNA was not detected until 80 to 100 min postinfection.


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  		TABLE 2. Phage resistance profile of L. lactis MG1614 containing AbiE, AbiF, LlaJI, and pNP40 against phage sk1 and sk1.m (propagated on the LlaJI+ host) at 30° C


Figure 6
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  		FIG. 6. Intracellular sk1 DNA replication in MG1614 (A) and MG1614/pNP40 (B). (A) Lane 1 contains purified sk1 control DNA, whereas lanes 2 to 5 represent total DNA samples isolated at 0, 20, 40, and 60 min postinfection, respectively, as indicated above each lane. Lysis had initiated with this host after 40 min. (B) Lane 1 contains purified sk1 control DNA, whereas lanes 2 to 8 represent total DNA isolated at 0, 20, 40, 60, 80, 100, and 120 min postinfection, respectively, as indicated above each lane. No lysis was evident with this host during the course of the experiment.

A "scan" of pNP40 was performed by the construction of a deletion derivative (pNP40{Delta}Soe1) and multiple subclones (pORF1, pORF13, pNZ-6.2, pNZ-7, and pNZ-10), essentially encompassing the orf11-to-orf35 region, which, when examined for any (loss of) associated phage resistance phenotype, failed to reveal the presence of an as-yet-unidentified resistance system (see Table 1 and Materials and Methods). Therefore, the residual phage resistance phenotype associated with pNP40 could not be ascribed to any of the distinctive genetic determinant(s) characterized. This resistance may be attributable to synergistic enhancement of the characterized resistance systems rather than the presence of a fourth (penetration blocking) system, particularly since AbiE and AbiF have previously been implicated in such a enhancement phenotype (46). An examination of the phage resistance profiles of specific AbiE– and AbiF– deletion derivatives of pNP40 would be required to verify this suggestion.

Concluding remarks. Analysis of the sequence of the 64.9-kbp pNP40 plasmid has provided the genetic confirmation and localization of a number of previously described functions such as conjugation, cadmium resistance, nisin resistance, bacteriophage resistance, and replication. In addition, new determinants for cold shock resistance and DNA damage repair were identified and confirmed phenotypically.

Lactococcal plasmids such as pNP40 appear to endow their respective hosts with multiple biologically and biotechnologically important properties, many of which have been genetically characterized (47). The extent to which pNP40 is able to limit bacteriophage proliferation must surely be a reflection of the selective pressure to which this plasmid and associated host have been exposed. In conclusion, it would appear that relative to the sequenced lactococcal plasmids to date (47, 62), the magnitude of the genetic "arsenal" possessed by pNP40 to cope with environmental hazards (some of which are unique to this plasmid, e.g., recALP, uvrA, abiEi, abiEii, LlaJI, and abiF) is particularly significant.


Figure 4
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  		FIG. 4— Continued.


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ACKNOWLEDGMENTS
 
This study was funded by Science Foundation Ireland (02/IN1/B198).

We thank Paul O'Toole and Stephen McGrath for helpful discussions.


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FOOTNOTES
 
* Corresponding author. Mailing address: Department of Microbiology, University College Cork, Western Road, Cork, Ireland. Phone: 353 214901365. Fax: 353 214903101. E-mail: d.vansinderen{at}ucc.ie. Back

{dagger} Supplemental material for this article may be found at http://jb.asm.org/. Back


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Journal of Bacteriology, September 2006, p. 6629-6639, Vol. 188, No. 18
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