Skip to main page content

• HOME
• Current Issue
• Archive
• Alerts
• About ASM
• Contact us
• Tech Support
• Journals.ASM.org

This Article Abstract Full Text (PDF) An erratum has been published Alert me when this article is cited Alert me if a correction is posted Services Similar articles in this journal Similar articles in PubMed Alert me to new issues of the journal Download to citation manager Reprints and Permissions Copyright Information Books from ASM Press MicrobeWorld Citing Articles Citing Articles via HighWire Citing Articles via Google Scholar Google Scholar Articles by Deveau, H. Articles by Moineau, S. Search for Related Content PubMed PubMed Citation Articles by Deveau, H. Articles by Moineau, S. Agricola Articles by Deveau, H. Articles by Moineau, S.

 Previous Article  |  Next Article 

Applied and Environmental Microbiology, September 2002, p. 4364-4369, Vol. 68, No. 9
0099-2240/02/$04.00+0     DOI: 10.1128/AEM.68.9.4364-4369.2002
Copyright © 2002, American Society for Microbiology. All Rights Reserved.

Effect of Exopolysaccharides on Phage-Host Interactions in Lactococcus lactis

Hélène Deveau,¹ Marie-Rose Van Calsteren,² and Sylvain Moineau^1*

Département de Biochimie et de Microbiologie, Faculté des Sciences et de Génie, Groupe de Recherche en Écologie Buccale (GREB), Faculté de Médecine Dentaire, Université Laval, Québec, Canada G1K 7P4,¹ Food Research and Development Centre, Agriculture and Agri-Food Canada, Saint-Hyacinthe, Québec, Canada J2S 8E3²

Received 29 January 2002/ Accepted 25 June 2002

Top Abstract Introduction Materials and Methods Results and Discussion References

 
In this study, we report that Lactococcus lactis strains producing exopolysaccharides (EPS) are sensitive to virulent phages. Eight distinct lytic phages (Q61 to Q68) specifically infecting Eps⁺ strains were isolated in 47 buttermilk samples obtained from 13 North American factories. The eight phages were classified within the 936 species by the multiplex PCR method, indicating that these phages are not fundamentally distinct from those infecting Eps^- L. lactis strains. The host range of these phages was determined with 19 Lactococcus strains, including 7 Eps⁺ and 12 Eps^- cultures. Three phages (Q62, Q63, and Q64) attacked only the Eps⁺ strain SMQ-419, whereas the five other phages (Q61, Q65, Q66, Q67, and Q68) infected only the Eps⁺ strain SMQ-420. The five other Eps⁺ strains (H414, MLT2, MLT3, SMQ-461, and SMQ-575) as well as the 12 Eps^- strains were insensitive to these phages. The monosaccharide composition of the polymer produced by the seven Eps⁺ strains was determined. The EPS produced by strains MLT3, SMQ-419, and SMQ-575 contained glucose, galactose, and rhamnose. The EPS fabricated by H414 contained only galactose. The EPS made by MLT2, SMQ-420, and SMQ-461 contained glucose and galactose. These findings indicate that the sugar composition of the EPS has no effect on phage sensitivity. The plasmid encoding the eps operon was cured from the two phage-sensitive strains. The cured derivatives were still phage sensitive, which indicates that EPS are not necessary for phage infection. Phage adsorption assays showed that the production of EPS does not confer a significant phage resistance phenotype.

Top Abstract Introduction Materials and Methods Results and Discussion References

 
Lactococcus lactis is a gram-positive lactic acid bacterium (LAB) used to acidify milk during the manufacture of fermented dairy products. Most Lactococcus strains contain numerous plasmids that encode key industrial phenotypes, including the production of extracellular polysaccharides (EPS). When produced in situ, these loosely bound exopolysaccharides decrease the syneresis, increase the viscosity, and improve the texture of dairy products. From a microbiological standpoint, EPS may also protect the producing cells against detrimental environmental conditions. The lactococcal EPS are heteropolysaccharides composed of repeating units of sugars in which galactose, glucose, and rhamnose are the most common carbohydrates. The structure and composition of several lactococcal EPS, as well as the sequence and organization of the eps genes, have also been resolved during the last decade (10, 13, 24, 34, 35, 36).

Lytic phages are the most significant cause of fermentation failures in the dairy industry worldwide (21). Lactococcal phages are currently classified into 12 distinct species (16), although a reduction to 11 species was recently proposed (18). However, only three species are predominant in most dairy plants: 936, c2, and P335 (3, 16-18, 22, 23). These three species are members of the Siphoviridae family and share some important features, including a double-stranded DNA genome and a long noncontractile tail (1, 16). The EPS-producing Lactococcus strains are increasingly used in the dairy industry, and it is well documented that extensive use of a particular strain will lead to milk fermentation failures due to virulent bacteriophages. Yet, to our knowledge, there are only two studies in the literature that mention lactococcal phages infecting EPS-producing strains (28, 31). In fact, a total of only three phages were described in these two studies conducted in the 1970s. The first study described the isolation of phages sl60 and sl122, but unfortunately, they were not characterized further (31). The second study described the isolation of phage KSY1, which belongs to the Podoviridae family, from the Finnish fermented milk called "viili" (28). KSY1 is the reference phage of the lactococcal phage species that bears its name. This morphotype is very rare, because only two KSY1-like phages have been reported in lactococci (28, 29). These results suggested that the lactococcal phages infecting EPS-producing strains may be different from those infecting non-EPS-producing strains, which are traditionally used in the manufacture of most fermented dairy products.

In the mid-1980s, Saxelin et al. (29) isolated and characterized by electron microscopy and host range 13 morphological types of phages from viili. However, it is not known whether these phages infected EPS-producing strains (29). Moineau et al. (22) showed that none of the 27 distinct lactococcal phages isolated from North American buttermilk factories could propagate on six EPS-producing strains. These results suggested that EPS production could protect cells against lytic phage infection (22). In fact, a number of authors have suggested that EPS may protect LAB against phages (7, 10, 12, 19, 22, 37). Looijesteijn et al. (19) demonstrated that cell-associated EPS granted lactococcal strains a slight protection against phages. Forde and Fitzgerald (12) revealed that loosely bound EPS produced by some Lactococcus strains partially inhibited phage adsorption, possibly by masking phage receptors. However, today, some EPS-producing lactococcal strains appear to be infected by phages in commercial applications such as buttermilk. Thus, the involvement of EPS in the phage infection process of LAB is still unclear.

In gram-negative bacteria, EPS and/or capsular polysaccharide may be directly involved in phage-host interactions. Specific phages infecting Escherichia coli and Vibrio cholerae strains that possess polysaccharide capsule have been isolated (2, 8, 30). In Rhizobium meliloti, the EPS production has been shown to inhibit phage adsorption (9).

The aim of this study was to characterize bacteriophages specifically infecting EPS-producing L. lactis strains and to study the effect of EPS on phage-host interactions.

Top Abstract Introduction Materials and Methods Results and Discussion References

 
Bacterial strains and media.
The L. lactis strains used in this study are listed in Table 1 and were grown at 30°C in M17 broth (32) supplemented with 0.5% glucose (GM17) or lactose (LM17) (Quélab, Montréal, Québec, Canada). The species and subspecies of lactococcal strains were confirmed as outlined previously (3, 26) with the reference strains L. lactis subsp. cremoris SMQ-5, L. lactis subsp. lactis IL-1403, and Streptococcus thermophilus SMQ-301. The seven Eps⁺ strains were genotypically identified as L. lactis subsp. cremoris.

View this table: [in this window] [in a new window]

TABLE 1. Bacterial strains and bacteriophages used in this study

Phage isolation and classification.
Forty-seven phage-containing samples from 13 North American buttermilk factories were provided by Quest International. The presence of phages in these samples was confirmed by spot test on seven EPS-producing Lactococcus strains as described elsewhere (22, 23). For each sample, five well-defined plaques were isolated, and high phage titers were obtained by the method of Jarvis (15). This procedure was repeated twice. The newly isolated phages were designated with the prefix "Q." All phages used in this study are listed in Table 1. These newly isolated lactococcal phages were classified within a phage species by the multiplex PCR method (17). Phage P008 was used as the reference for the 936 species, phage c2 was used as the reference for the c2 species, and phage P335 was used as the reference for the P335 species. Phage morphology was observed with a Phillips 420 transmission electron microscope at 80 kV as described previously (23). The host range of the isolated phages was determined on 19 industrial L. lactis strains, which included 7 EPS-producing strains (Eps⁺) and 12 EPS-negative strains (Eps^-), as described previously (23).

Phage DNA isolation.
The Maxi Lambda DNA purification kit (Qiagen, Chatsworth, Calif.) was used for lactococcal phage DNA purification with the following modifications: L2 buffer was adjusted to provide a final concentration of 10% polyethylene glycol and 0.5 M sodium chloride. Proteinase K (100 µl of a 20-mg/ml solution) was added before the L4 buffer. The mixture was incubated for 30 min at 55°C. DNA was resuspended in 100 µl of 10 mM Tris-HCl (pH 7.8) and stored at -20°C for later use.

DNA manipulations.
Plasmid DNA was purified by the modified method of O'Sullivan and Klaenhammer (25). Total DNA of L. lactis strains was extracted by the method described by Hill et al. (14) with some modifications. The Tris-EDTA (TE)-saturated phenol was replaced by two steps involving an equal volume of phenol-chloroform. One-fifth volume of 7.5 M ammonium acetate was added, and the DNA was precipitated by the addition of 2 volumes of cold 95% ethanol. Restriction endonucleases (Roche Diagnostics, Laval, Québec, Canada) were used as recommended by the manufacturer. After restriction, phage DNA samples were heated for 10 min at 70°C to avoid possible cohesive end ligation. DNA was electrophoresed on 0.8% agarose gels in 1x TAE buffer (40 mM Tris-acetate, 1 mM EDTA) and visualized by UV photography after staining in ethidium bromide.

Analysis of EPS composition.
For each strain, 1 liter of LM17 was inoculated with an overnight culture (1% [vol/vol]) and incubated at 25°C for 48 h. The EPS was extracted by the method of Cerning (6) and further purified on a Sephacryl S-400 HR column by elution with 50 mM NH₄HCO₃. The polymer (1 mg) was hydrolyzed (2 M trifluoroacetic acid, 1 h, 121°C) and analyzed by high-performance liquid chromatography (HPLC) at 65°C on a 30-cm by 7.8-mm Aminex-87H column (Bio-Rad, Mississauga, Ontario, Canada), eluted at 0.6 ml/min with 0.005 N sulfuric acid. The sugars were detected by refractive index monitoring at 35°C.

Plasmid curing and microbiological assays.
The L. lactis Eps⁺ strains SMQ-419 and SMQ-420 were cured of the plasmid containing the eps operon by serial transfers in GM17 broth. After 1 week, the culture was streaked, and isolated colonies were transferred in milk and incubated for 16 h at 25°C. Strains were regarded as ropy if strings of 5 mm or more were detected when the culture was touched with a sterile pipette. The plasmid and total DNA of nonmucoid isolates were extracted, and the absence or presence of the eps gene cluster was verified by Southern analysis. Efficiency of plating was performed on Eps^- and Eps⁺ isolates as described previously (27). Phage adsorption tests were carried out on the L. lactis strains SMQ-419, SMQ-420, SMQ-737, and SMQ-738, as described previously (11), but with the following modifications: GM17 broth was used, and the incubation temperature was 30°C. Phage adsorption assays were also performed on bacterial cells washed twice with 0.1% peptone (9).

Detection of the eps gene cluster.
Plasmid and chromosomal DNAs were transferred onto positively charged nylon membranes by capillary blotting. The probe was constructed by labeling PCR fragments with the Dig High-Prime labeling kit (Roche). The probe was made of a PCR product corresponding to the epsD (priming glycosyltransferase) gene (primers 5'-TGATCCCCGTGTAACGAAGA-3' and 5'-AAGAGAGGCGCTCCCCATAT-3'). Prehybridization, hybridization, washes, and detection by chemiluminescence were performed as suggested by the manufacturer (Roche).

Top Abstract Introduction Materials and Methods Results and Discussion References

 
Phage isolation.
The phage content of 47 buttermilk samples from 13 dairy manufacturing plants was examined by analyzing a total of 235 single plaques (5 plaques per sample) propagated on EPS-producing L. lactis strains. Based on DNA restriction profiles with EcoRV (Fig. 1) and EcoRI (data not shown), only eight different phages were found among the 235 isolates. Furthermore, some of these phages were very similar. Only one phage was isolated from the samples provided by four factories. In the nine remaining factories, between two and four different lactococcal phages were found. A buttermilk manufacturing facility can therefore harbor many distinct phages. Phages with identical DNA restriction profiles were also detected in many factories. For example, phage Q67 was isolated in six factories and Q64 was found in 8 of 13 dairies, indicating that a specific phage can be found in several geographic locations. Three phages (Q63, Q66, and Q68) were unique to one plant. The isolation of multiple lactococcal phages within one plant was not surprising, because a similar phenomenon was previously observed in cheese plants (3). Because these facilities used similar and application-oriented starter cultures and the use of specific strains will partly dictate the presence of particular phages within a dairy plant, these eight phages appear fit to propagate under the buttermilk manufacturing conditions. These results also unequivocally showed that EPS-producing lactococcal strains can be infected by phages during buttermilk production.

View larger version (1K): [in this window] [in a new window]

FIG. 1. Characterization of lactococcal phages Q61 to Q68. (A) Dendrogram of EcoRV restriction profiles of the eight lactococcal phages. (B) Classification of the eight phages by multiplex PCR.

Phage classification.
The multiplex PCR method was performed to catalogue the eight newly isolated phages within the three most common lactococcal phage species found in dairy plants, namely, 936, c2, and P335 (17, 21). The eight phages isolated in this study gave a PCR product slightly lower than 200 bp, indicating that they all belong to the species 936 (Fig. 1). The typical 936 morphology (isometric head and noncontractile tail) was confirmed by electron microscopy (data not shown). These results indicate that these phages are not fundamentally distinct from those infecting Eps^- L. lactis strains. They also suggest that the previous isolation of phages from the KSY1 species may indeed be a very rare event (28, 29).

Host range.
The host range of the eight phages was determined on 19 lactococcal strains, which included 7 Eps⁺ strains and 12 Eps^- strains. These strains are currently used in various combinations within several commercial starter cultures (3 strains per starter) for buttermilk production. All 12 Eps^- strains were insensitive to the eight phages. Only two of seven mucoid strains were sensitive to these phages (Table 2). L. lactis SMQ-419 was sensitive to phages Q62, Q63, and Q64, whereas L. lactis SMQ-420 was sensitive to phages Q61, Q65, Q66, Q67, and Q68. These results show that the eight phages are specific to two Eps⁺ L. lactis strains.

View this table: [in this window] [in a new window]

TABLE 2. Classification of EPS produced by seven strains and phage sensitivity of these strains

Analysis of the EPS composition.
The EPS produced by the seven EPS-producing strains was purified, hydrolyzed, and analyzed by HPLC for their monosaccharide composition. The L. lactis Eps⁺ strains MLT3 (group I), H414 (group II), and MLT2 (group III) were used as reference strains in accordance with the classification of van Kranenburg et al. (36). The monosaccharide composition of the EPS produced by the three reference strains was in agreement with those reported in the literature (36). The EPS produced by strains MLT3, SMQ-419, and SMQ-575 (group I) contained glucose, galactose, and rhamnose (Table 2). The EPS fabricated by strain H414 (group II) contained only galactose. The EPS made by strains MLT2 and SMQ-420 (group III) contained glucose and galactose. The EPS assembled by strain SMQ-461 also contained only glucose and galactose, but preliminary nuclear magnetic resonance analysis showed that the structure of this EPS is different from the one produced by group III, and it may belong to another group (data not shown). Given that phage-sensitive and phage-insensitive strains were found to produce EPS that belong to either group I (glucose, galactose, and rhamnose) or group III (glucose and galactose), these results clearly indicate that the monosaccharide composition of the EPS has no influence on the phage sensitivity of an L. lactis strain.

Effect of EPS on phage sensitivity.
The phage-sensitive strains SMQ-419 and SMQ-420 were cured of the plasmid coding for the EPS production, and the cured derivatives were named SMQ-737 and SMQ-738, respectively. The absence of these plasmids in the cured derivatives was verified by plasmid profile analysis, and the absence of the eps operon was confirmed by Southern analysis in which an epsD (priming glycosyltransferase) probe failed to hybridize with total DNA (data not shown). Both cured derivatives exhibited the same phage sensitivity as that of their parents, indicating that the EPS is not necessary for phage infection. The efficiency of plating (EOP; phage titer on the Eps⁺ strain divided by the phage titer on the Eps^- strain) of these phages was also measured (Table 3). The EOP of phages Q61, Q65, Q66, Q67 and Q68 were 1.0, indicating the plasmid encoding the eps operon in L. lactis SMQ-420 does not confer a phage resistance phenotype. By association, these data also indicated that the EPS produced by SMQ-420 (containing glucose and galactose) does not prevent phage infection. The EOP of phages Q62 and Q63 were slightly below 1.0, indicating that the plasmid encoding the eps operon in L. lactis SMQ-419 may arguably provide weak resistance against these two phages. This limited antiviral phenotype is likely due to the production of the EPS (containing glucose, galactose, and rhamnose).

View this table: [in this window] [in a new window]

TABLE 3. EOP of phages Q61 to Q68 on L. lactis SMQ-737 and SMQ-738

Effect of EPS on phage adsorption.
The percentages of phage adsorption on wild-type strains (Eps⁺) and cured derivatives (Eps^-) were compared. No significant differences were observed between the phage adsorption on SMQ-420 (Eps⁺) and that on SMQ-738 (Eps^-) (data not shown). The adsorption of phages Q62, Q63, and Q64 was somewhat better on the SMQ-737 strain (Eps^-) than on the parent Eps⁺ strain SMQ-419 (Table 4). The standard deviations were relatively high (13 to 15%) for the phage adsorption results with the Eps⁺ strain L. lactis SMQ-419 compared to similar data from the Eps^- strain SMQ-737 (0.6 to 4%). When the cells were washed to remove the loosely bound EPS, the percentages of phage adsorption were similar on both strains, and the standard deviations were lower (between 3.6 and 5.0%) (Table 4). The variability in the phage adsorption assays may be explained by the fluctuating EPS production. These results indicate that the EPS is likely responsible for the difference between the adsorption on SMQ-419 and that on SMQ-737. Moreover, these data confirm that the weak resistance against phages Q62 and Q63 is conferred by the EPS. These results are in agreement with those of Looijesteijn et al. (19), which showed that the production of group I EPS (such as those produced by SMQ-419) confers a marginal phage resistance phenotype (EOP above 0.5).

View this table: [in this window] [in a new window]

TABLE 4. Adsorption percentage of phages Q62, Q63, and Q64 on L. lactis SMQ-419 and SMQ-737

The production of EPS increases the viscosity of the medium, and perhaps this molecular crowding slightly affects the spread of phage infection. It also possible that the EPS could protect the strain by coating the cell, but this protection would be limited because the lactococcal EPS is loosely bound. Nonetheless, it is clear from the evidence presented above that processors should not rely on the production of EPS to protect starter cultures against phages. It remains to be seen if the structure of some lactococcal EPS could be involved in phage sensitivity or insensitivity. Finally, the mine if other phage resistance mechanisms are present in the phage-insensitive Eps⁺ strains. Finally, the phage insensitivity reported here may simply be related to the absence of specific phage receptors on the cell surface of these strains. Further research is under way to address these issues. To our knowledge, this is the first thorough analysis of phages infecting EPS-producing gram-positive bacteria.

 
We are grateful to Quest International for providing buttermilk samples and to R. van Kranenburg for strains MLT2 and MLT3. We thank J. Bouchard, S. Labrie, D. Roy, and D. Tremblay for helpful discussions. We also thank C. B. Do, C. Danis, and A. Bégin for help during EPS purification and for sugar analysis, as well as D. Montpetit for electron microscopy.

We thank the NSERC (Research Network on LAB), Agriculture and Agri-Food Canada, Novalait, Inc., Dairy Farmers of Canada, and Institut Rosell-Lallemand, Inc., for financial support. H.D. is a recipient of a Fonds FCAR graduate scholarship.

 
* Corresponding author. Mailing address: Groupe de Recherche en Écologie Buccale (GREB), Faculté de Médecine Dentaire, Université Laval, Québec, Canada G1K 7P4. Phone: 418-656-3712. Fax: 418-656-2861. E-mail: Sylvain.Moineau{at}bcm.ulaval.ca.

Top Abstract Introduction Materials and Methods Results and Discussion References

 

1
1. Ackermann, H.-W., E. D. Cantor, A. W. Jarvis, J. Lembke, and J. A. Mayo. 1984. New species definitions in phages of Gram-positive cocci. Intervirology 22:181-190.[Medline]
2
2. Albert, M. J., N. A. Bhuiyan, A. Rahman, A. N. Ghosh, K. Hultenby, A. Weintraub, S. Nahar, A. K. M. G. Kibriya, M. Ansaruzzaman, and T. Shimada. 1996. Phage specific for Vibrio cholerae O139 Bengal. J. Clin. Microbiol. 34:1843-1845.[Abstract]
3
3. Bissonnette, F., S. Labrie, H. Deveau, M. Lamoureux, and S. Moineau. 2000. Characterization of mesophilic mixed starter cultures used for the manufacture of aged cheddar cheese. J. Dairy Sci. 83:620-627.[Abstract]
4
4. Bolotin, A., P. Wincker, S. Mauger, O. Jaillon, K. Malarme, J. Weissenbach, S. D. Ehrlich, and A. Sorokin. 2001. The complete genome sequence of the lactic acid bacterium Lactococcus lactis ssp. lactis IL1403. Genome Res. 11:731-753.
5
5. Braun, V., S. Hertwig, H. Neve, A. Geis, and M. Teuber. 1989. Taxonomic differentiation of bacteriophages of Lactococcus lactis by electron microscopy, DNA-DNA hybridization, and protein profiles. J. Gen. Microbiol. 135:2551-2560.
6
6. Cerning, J. 1990. Exocellular polysaccharides produced by lactic acid bacteria. FEMS Microbiol. Lett. 87:113-130.[CrossRef]
7
7. Cerning, J. 1995. Production of exopolysaccharides by lactic acid bacteria and dairy propionibacteria. Lait 75:463-472.
8
8. Clarke, B. R., F. Esumeh, and I. S. Roberts. 2000. Cloning, expression, and purification of the K5 capsular polysaccharide lyase (KflA) from coliphage K5A: evidence for two distinct K5 lyase enzymes. J. Bacteriol. 182:3761-3766.[Abstract/Free Full Text]
9
9. Defives, C., M. Werquin, P. Mary, and J. P. Hormez. 1996. Roles of exopolysaccharides and lipopolysaccharides in the adsorption of the Siphovirus phage NM8 to Rhizobium meliloti M11S cells. Curr. Microbiol. 33:371-376.[CrossRef][Medline]
10
10. De Vuyst, L., and B. Degeest. 1999. Heteropolysaccharides from lactic acid bacteria. FEMS Microbiol. Rev. 23:153-177.[CrossRef][Medline]
11
11. Duplessis, M., and S. Moineau. 2001. Identification of a genetic determinant responsible for the host specificity in Streptococcus thermophilus bacteriophages. Mol. Microbiol. 41:325-336.[CrossRef][Medline]
12
12. Forde, A., and G. F. Fitzgerald. 1999. Analysis of exopolysaccharide (EPS) production mediated by the bacteriophage adsorption blocking plasmid, pCI658, isolated from Lactococcus lactis ssp. cremoris HO2. Int. Dairy J. 9:465-472.[CrossRef]
13
13. Gruter, M., B. R. Leeflang, J. Kuiper, J. P. Kamerling, and J. F. G. Vliegenthart. 1992. Structure of the exopolysaccharide produced by Lactococcus lactis subspecies cremoris H414 grown in a defined medium or skimmed milk. Carbohydr. Res. 231:273-291.[CrossRef][Medline]
14
14. Hill, C., J. Massey, and T. R. Klaenhammer. 1991. Rapid method to characterize lactococcal bacteriophage genomes. Appl. Environ. Microbiol. 57:283-288.[Abstract/Free Full Text]
15
15. Jarvis, A. W. 1978. Serological studies of a host range mutant of a lactic streptococcal bacteriophage. Appl. Environ. Microbiol. 36:785-789.[Abstract/Free Full Text]
16
16. Jarvis, A. W., G. F. Fitzgerald, M. Mata, A. Mercenier, H. Neve, I. B. Powell, C. Ronda, M. Saxelin, and M. Teuber. 1991. Species and type phages of lactococcal bacteriophages. Intervirology 32:2-9.[Medline]
17
17. Labrie, S., and S. Moineau. 2000. Multiplex PCR for detection and identification of lactococcal bacteriophages. Appl. Environ. Microbiol. 66:987-994.[Abstract/Free Full Text]
18
18. Labrie, S., and S. Moineau. 2001. Complete genomic sequence of bacteriophage ul36: demonstration of phage heterogeneity within the P335 quasi-species of lactococcal phages. Virology 296:308-320.
19
19. Looijesteijn, P. J., L. Trapet, E. de Vries, T. Abee, and J. Hugenholtz. 2001. Physiological function of exopolysaccharides produced by Lactococcus lactis. Int. J. Food Sci. 64:71-80.
20
20. McKay, L. L., K. A. Baldwin, and E. A. Zottola. 1972. Loss of lactose metabolism in lactic streptococci. Appl. Microbiol. 23:1090-1096.[Medline]
21
21. Moineau, S. 1999. Applications of phage resistance in lactic acid bacteria. Antonie Leeuwenhoek 76:377-382.
22
22. Moineau, S., M. Borkaev, B. J. Holler, S. A. Walker, J. K. Kondo, E. R. Vedamuthu, and P. A. Vanderbergh. 1996. Isolation and characterization of lactococcal bacteriophages from cultured buttermilk plants in the United States. J. Dairy Sci. 79:2104-2111.[Abstract]
23
23. Moineau, S., J. Fortier, H.-W. Ackermann, and S. Pandian. 1992. Characterization of lactococcal bacteriophages from Quebec cheese plants. Can. J. Microbiol. 38:875-882.
24
24. Nakajima, H., S. Toyoda, T. Toba, T. Itoh, T. Mukai, H. Kitazawa, and S. Adachi. 1990. A novel phosphopolysaccharide from slime-forming Lactococcus lactis subspecies cremoris SBT 0495. J. Dairy Sci. 73:1472-1477.[Abstract]
25
25. O'Sullivan, D. J., and T. R. Klaenhammer. 1993. Rapid mini-prep isolation of high-quality plasmid DNA from Lactococcus and Lactobacillus spp. Appl. Environ. Microbiol. 59:2730-2733.[Abstract/Free Full Text]
26
26. Salama, M., W. Sandine, and S. Giovannoni. 1991. Development and application of oligonucleotide probes for identification of Lactococcus lactis subsp. cremoris. Appl. Environ. Microbiol. 57:1313-1318.
27
27. Sanders, M. E., and T. R. Klaenhammer. 1980. Restriction and modification in group N streptococci: effect of heat on development of modified lytic bacteriophage. Appl. Environ. Microbiol. 40:500-506.[Abstract/Free Full Text]
28
28. Saxelin, M.-L., E.-L. Nurmiaho, M. P. Korhola, and V. Sundman. 1979. Partial characterization of a new C3-type capsule-dissolving phage of Streptococcus cremoris. Can. J. Microbiol. 25:1182-1187.[Medline]
29
29. Saxelin, M.-L., E.-L. Nurmiaho-Lassila, V. T. Meriläinen, and R. I. Forsén. 1986. Ultrastructure and host specificity of bacteriophages of Streptococcus cremoris, Streptococcus lactis subsp. diacetylactis, and Leuconostoc cremoris from Finnish fermented milk "viili." Appl. Environ. Microbiol. 52:771-777.[Abstract/Free Full Text]
30
30. Scholl, D., S. Rogers, S. Adhya, and C. R. Merril. 2001. Bacteriophage K1-5 encodes two different tail fiber proteins, allowing it to infect and replicate on both K1 and K5 strains of Escherichia coli. J. Virol. 75:2509-2515.[Abstract/Free Full Text]
31
31. Sozzi, T., J. M. Poulin, R. Maret, and R. Pousaz. 1978. Isolation and some characteristics of phages of ropy strains of Streptococcus lactis. Milchwissenschaft 33:349-352.
32
32. Terzaghi, B. E., and W. E. Sandine. 1975. Improved medium for lacticstreptococci and their bacteriophages. Appl. Microbiol. 29:807-813.
33
33. Tremblay, D. M., and S. Moineau. 1999. Complete genomic sequence of the lytic bacteriophage DT1 of Streptococcus thermophilus. Virology 255:63-76.[CrossRef][Medline]
34
34. van Casteren, W. H. M., P. de Waard, C. Dijkema, H. A. Schols, and A. G. J. Voragen. 2000. Structural characterisation and enzymatic modification of the exopolysaccharide produced by Lactococcus lactis subsp. cremoris B891. Carbohydr. Res. 327:411-422.
35
35. van Casteren, W. H. M., C. Dijkema, H. A. Schols, G. Beldman, and A. G. J. Voragen. 2000. Structural characterisation and enzymatic modification of the exopolysaccharide produced by Lactococcus lactis subsp. cremoris B39. Carbohydr. Res. 324:170-181.
36
36. van Kranenburg, R., H. R. Vos, I. I. van Swam, M. Kleerebezem, and W. M. de Vos. 1999. Functional analysis of glycosyltransferase genes from Lactococcus lactis and other gram-positive cocci: complementation, expression, and diversity. J. Bacteriol. 181:6347-6353.[Abstract/Free Full Text]
37
37. Vedamuthu, E. R., and J. M. Neville. 1986. Involvement of a plasmid in production of ropiness (mucoidness) in milk cultures by Streptococcus cremoris MS. Appl. Environ. Microbiol. 51:677-682.[Abstract/Free Full Text]

---

Applied and Environmental Microbiology, September 2002, p. 4364-4369, Vol. 68, No. 9
0099-2240/02/$04.00+0     DOI: 10.1128/AEM.68.9.4364-4369.2002
Copyright © 2002, American Society for Microbiology. All Rights Reserved.

This article has been cited by other articles:

• Rousseau, G. M., Moineau, S. (2009). Evolution of Lactococcus lactis Phages within a Cheese Factory. Appl. Environ. Microbiol. 75: 5336-5344 [Abstract] [Full Text]  
• Siponen, M., Spinelli, S., Blangy, S., Moineau, S., Cambillau, C., Campanacci, V. (2009). Crystal Structure of a Chimeric Receptor Binding Protein Constructed from Two Lactococcal Phages. J. Bacteriol. 191: 3220-3225 [Abstract] [Full Text]  
• Briandet, R., Lacroix-Gueu, P., Renault, M., Lecart, S., Meylheuc, T., Bidnenko, E., Steenkeste, K., Bellon-Fontaine, M.-N., Fontaine-Aupart, M.-P. (2008). Fluorescence Correlation Spectroscopy To Study Diffusion and Reaction of Bacteriophages inside Biofilms. Appl. Environ. Microbiol. 74: 2135-2143 [Abstract] [Full Text]  
• Deveau, H., Barrangou, R., Garneau, J. E., Labonte, J., Fremaux, C., Boyaval, P., Romero, D. A., Horvath, P., Moineau, S. (2008). Phage Response to CRISPR-Encoded Resistance in Streptococcus thermophilus. J. Bacteriol. 190: 1390-1400 [Abstract] [Full Text]  
• Deveau, H., Labrie, S. J., Chopin, M.-C., Moineau, S. (2006). Biodiversity and classification of lactococcal phages.. Appl. Environ. Microbiol. 72: 4338-4346 [Abstract] [Full Text]  
• Spinelli, S., Campanacci, V., Blangy, S., Moineau, S., Tegoni, M., Cambillau, C. (2006). Modular Structure of the Receptor Binding Proteins of Lactococcus lactis Phages: THE RBP STRUCTURE OF THE TEMPERATE PHAGE TP901-1. J. Biol. Chem. 281: 14256-14262 [Abstract] [Full Text]  
• Tremblay, D. M., Tegoni, M., Spinelli, S., Campanacci, V., Blangy, S., Huyghe, C., Desmyter, A., Labrie, S., Moineau, S., Cambillau, C. (2006). Receptor-Binding Protein of Lactococcus lactis Phages: Identification and Characterization of the Saccharide Receptor-Binding Site.. J. Bacteriol. 188: 2400-2410 [Abstract] [Full Text]  
• Dabour, N., LaPointe, G. (2005). Identification and Molecular Characterization of the Chromosomal Exopolysaccharide Biosynthesis Gene Cluster from Lactococcus lactis subsp. cremoris SMQ-461. Appl. Environ. Microbiol. 71: 7414-7425 [Abstract] [Full Text]  
• Levesque, C., Duplessis, M., Labonte, J., Labrie, S., Fremaux, C., Tremblay, D., Moineau, S. (2005). Genomic Organization and Molecular Analysis of Virulent Bacteriophage 2972 Infecting an Exopolysaccharide-Producing Streptococcus thermophilus Strain. Appl. Environ. Microbiol. 71: 4057-4068 [Abstract] [Full Text]  
• Deveau, H., Moineau, S. (2003). Technical Note: Use of RFLP to Characterize Lactococcus lactis Strains Producing Exopolysaccharides. J DAIRY SCI 86: 1472-1475 [Abstract] [Full Text]  
• Broadbent, J. R., McMahon, D. J., Welker, D. L., Oberg, C. J., Moineau, S. (2003). Biochemistry, Genetics, and Applications of Exopolysaccharide Production in Streptococcus thermophilus: A Review. J DAIRY SCI 86: 407-423 [Abstract] [Full Text]  

This Article Abstract Full Text (PDF) An erratum has been published Alert me when this article is cited Alert me if a correction is posted Services Similar articles in this journal Similar articles in PubMed Alert me to new issues of the journal Download to citation manager Reprints and Permissions Copyright Information Books from ASM Press MicrobeWorld Citing Articles Citing Articles via HighWire Citing Articles via Google Scholar Google Scholar Articles by Deveau, H. Articles by Moineau, S. Search for Related Content PubMed PubMed Citation Articles by Deveau, H. Articles by Moineau, S. Agricola Articles by Deveau, H. Articles by Moineau, S.