Quantitative determination by real-time PCR of four vaginal Lactobacillus species , Gardnerella vaginalis and Atopobium vaginae indicates an inverse relationship between L. gasseri and L. iners

Ellen De Backer; Rita Verhelst; Hans Verstraelen; Mohammed A Alqumber; Jeremy P Burton; John R Tagg; Marleen Temmerman; Mario Vaneechoutte

doi:10.1186/1471-2180-7-115

Research article

Open Access

Quantitative determination by real-time PCR of four vaginal Lactobacillus species, Gardnerella vaginalis and Atopobium vaginae indicates an inverse relationship between L. gasseri and L. iners

Ellen De Backer¹,
Rita Verhelst¹,
Hans Verstraelen²,
Mohammed A Alqumber³,
Jeremy P Burton⁴,
John R Tagg³,
Marleen Temmerman² and
Mario Vaneechoutte¹Email author

BMC Microbiology20077:115

https://doi.org/10.1186/1471-2180-7-115

Received: 08 August 2007

Accepted: 19 December 2007

Published: 19 December 2007

Abstract

Background

Most studies of the vaginal microflora have been based on culture or on qualitative molecular techniques. Here we applied existing real-time PCR formats for Lactobacillus crispatus, L. gasseri and Gardnerella vaginalis and developed new formats for Atopobium vaginae, L. iners and L. jensenii to obtain a quantitative non culture-based determination of these species in 71 vaginal samples from 32 pregnant and 28 non-pregnant women aged between 18 and 45 years.

Results

The 71 vaginal microflora samples of these women were categorized, using the Ison and Hay criteria, as refined by Verhelst et al. (2005), as follows: grade Ia: 8 samples, grade Iab: 10, grade Ib: 13, grade I-like: 10, grade II: 11, grade III: 12 and grade IV: 7.

L. crispatus was found in all but 5 samples and was the most frequent Lactobacillus species detected. A significantly lower concentration of L. crispatus was found in grades II (p < 0.0001) and III (p = 0.002) compared to grade I. L. jensenii was found in all grades but showed higher concentration in grade Iab than in grade Ia (p = 0.024). A. vaginae and G. vaginalis were present in high concentrations in grade III, with log₁₀ median concentrations (log₁₀ MC), respectively of 9.0 and 9.2 cells/ml. Twenty (38.5%) of the 52 G. vaginalis positive samples were also positive for A. vaginae. In grade II we found almost no L. iners (log₁₀ MC: 0/ml) but a high concentration of L. gasseri ( log₁₀ MC: 8.7/ml). By contrast, in grade III we found a high concentration of L. iners ( log₁₀ MC: 8.3/ml) and a low concentration of L. gasseri ( log₁₀ MC: 0/ml). These results show a negative association between L. gasseri and L. iners (r = -0.397, p = 0.001) and between L. gasseri and A. vaginae (r = -0.408, p < 0.0001).

Conclusion

In our study we found a clear negative association between L. iners and L. gasseri and between A. vaginae and L. gasseri. Our results do not provide support for the generally held proposition that grade II is an intermediate stage between grades I and III, because L. gasseri, abundant in grade II is not predominant in grade III, whereas L. iners, abundant in grade III is present only in low numbers in grade II samples.

Keywords

LactobacillusBacterial VaginosisMinimal Inhibitory ConcentrationTerminal Restriction Fragment Length PolymorphismLactobacillus Species

Background

Bacterial vaginosis (BV) is considered to be the most frequent vaginal infectious disorder in women of childbearing age. Prevalences of 4.9% to 36% have been reported from European and American studies [1]. The condition is symptomatic in half of the women and also represents a psychological burden. More importantly, this disturbed vaginal microflora can cause serious sequelae such as non-gonococcal, non-chlamydial PID (Pelvic Inflammatory Disease) [2, 3], postpartum endometritis [4] and preterm birth [5–7]. Indeed, 40% of the cases of spontaneous preterm labor and preterm birth are thought to be associated with BV [8]. BV has also been associated with increased susceptibility to HIV and to genital tract infection with Chlamydia trachomatis and Neisseria gonorrhoeae [9–11].

BV is characterized by an overgrowth of many different, mostly anaerobic, bacteria. Gardnerella vaginalis has been considered to be the most characteristic microorganism in BV, but its pathogenic role was unclear, until recently, when the establishment of bacterial biofilm as a potential cause of recurrent BV [12], with a predominant presence of G. vaginalis, has clearly established a pathogenic role for this bacterium. Also recently, Atopobium vaginae has been strongly associated with BV, independently by different groups [13–15] and with biofilm in BV [12]. The suggestion that its association with BV is stronger than that of G. vaginalis, basically because G. vaginalis is more frequently detected in a normal vaginal microflora than A. vaginae [14] was confirmed by more recent studies [16, 17]. The insight that biofilm is formed in BV [12] has strong explanatory power with regard to the high recurrence rate of BV, despite initial relief after antibiotic treatment [18] and is in perfect correlation with the presence of the characteristic cells or 'clue cells', which are vaginal epithelial cells covered with layers of bacteria.

Four species of lactobacilli are now considered to be predominantly linked to the vaginal microflora: Lactobacillus crispatus, L. jensenii, L. gasseri and L. iners, with the latter only recently being recognized as it was long overlooked because it does not grow on De Man Rogosa Sharpe agar, the medium typically used to culture lactobacilli [19, 20].

In 1983 Spiegel et al. [21] devised a method for the diagnosis of bacterial vaginosis by direct Gram stain. Nugent et al. [22] proposed a modification of these criteria. By counting the different cell types (Lactobacillus spp., Gardnerella vaginalis/Bacteroides spp., Mobiluncus spp.) a score between zero and ten is obtained, whereby a score of 7 or higher corresponds to bacterial vaginosis and a score between 3 and 7 is considered intermediate between undisturbed vaginal microflora and bacterial vaginosis. Ison and Hay [23] suggested a simplification of this time-consuming approach, through an estimation of the ratios of the observed cellular types rather than the determination of the exact number of the bacteria and distinguished five grades (0 (no bacteria), I (normal), II (intermediate), III (bacterial vaginosis) and IV (streptococci)). Verhelst et al. [24] recently suggested, on the basis of Gram stain, terminal restriction fragment length polymorphism analysis of the 16S rRNA gene (T-RFLP) and molecular identification (tDNA-PCR) of cultured isolates, a new classification of the undisturbed vaginal microflora (grade I) whereby grade I microflora could be split up into four categories, designated grade Ia, Ib, Iab and I-like. Grade Ia was shown to contain predominantly L. crispatus, grade Ib predominantly L. gasseri and L. iners, grade Iab a mixture of these three species and grade I-like Bifidobacterium spp. rather than Lactobacillus spp. Grade I-like microflora, of which the Gram stain at first glance indicates the presence of lactobacilli, was considered as not representative for normal vaginal micoflora, but as probably an unrecognized type of disturbed vaginal microflora [25] that had previously not been distinguished from a healthy vaginal microflora.

In this study, we developed real-time PCR primers for L. iners, L. jensenii and A. vaginae and used these, together with described real-time PCR formats for L. crispatus [26], L. gasseri [26] and G. vaginalis [27], in an attempt to quantify some of the important bacterial species in the normal and disturbed vaginal microflora.

Results

Grading of vaginal microflora

In this study, Gram-stained smears of 71 vaginal swabs from 60 women, 32 of whom were pregnant, were examined microscopically. For 11 pregnant women the Gram stain based grading of their vaginal microflora differed between two trimesters and therefore swabs from both trimesters were included. Eight women had a vaginal microflora categorized by Gram stain as grade Ia, 10 as grade Iab, 13 as grade Ib, 10 as grade I-like, 11 as grade II, 12 as grade III and 7 as grade IV, according to criteria described previously [24].

Primer development and real-time PCR format

Primers for real-time PCR for Atopobium vaginae, Lactobacillus iners and L. jensenii were developed during this study (Tables 1, 2, 3). Primer positions relative to the 16S rRNA gene of Escherichia coli are presented in Figure 1. Table 4 lists all primers used and the real-time PCR formats. No cross-reactivity was detected with DNA from any of the tested species, including closely-related Lactobacillus and Atopobium species. In addition we found no cross reactivity for Bifidobacterium bifidum, B. breve and B. infantis with the G. vaginalis primers developed by Zariffard et al. [27].

Figure 1
Localisation of the primers used in this study on the 16S rRNA gene.

Table 1

Alignment of the 16S rRNA gene primers of L. iners with the sequences of other important vaginal lactobacilli

Forward primer (position 70–85)	5'																			3'
L. iners		G	T	C	T	G	C	C	T	T	G	A	A	G	A	T	C	G	G
L. crispatus		A	C	.	.	.	.	.	C	C	A	T	.	.	T	C	T	.	.
L. gasseri		A	C	.	.	.	.	.	C	A	A	G	.	.		C	T	.	.
L. jensenii		A	C	.	.	.	.	.	C	.	T	.	.	.	T	C	T	.	.
L. vaginalis		A	C	.	.	.	.	.	C	.	.	.	.	.	C	G	G	.	.
Reverse primer (position 228–210)	5'																				3'
L. iners		A	C	A	G	T	T	G	A	T	A	G	G	C	A	T	C	A	T	C
L. crispatus		.	.	.	C	.	.	A	G	C	.	C	T	.	.	.	.	G	.	T
L. gasseri		.	.	.	C	.	.	A	G	C	.	C	T	.	.	.	.	G	.	T
L. jensenii		.	.	.	C	.	.	A	G	C	.	C	T	.	.	.	.	G	.	T
L. vaginalis		.	.	.	C	C	.	A	G	C	.	C	T	.	.	.	.	G	.	T

Table 2

Alignment of the 16S rRNA gene primers of L. jensenii, with the sequences of other important vaginal lactobacilli

Forward primer (position 117–137)	5'																						3'
L. jensenii		C	C	T	T	A	A	G	T	C	T	G	G	G	A	T	A	C	C	A	T	T
L. crispatus		.	.	C	A	T	.	.	.	.	.	.	.	.	.	.	.	.	.	.	C	.
L. gasseri		.	.	A	A	G	.	.	A	.	.	.	.	.	.	.	.	A	.	.	C	C
L. iners		.	.	A	A	G	.	.	A	T	C	.	.	.	.	.	.	A	.	.	C	C
L. vaginalis		.	.	.	G	.	.	.	C	G	G	.	.	.	.	.	.	A	.	.	.	C
Reverse primer (position 207–187)	5'																						3'
L. jensenii		A	C	G	C	C	G	C	C	T	T	T	T	A	A	A	C	T	T	C	T	T
L. crispatus		.	.	.	.	.	.	.	.	.	.	.	.	.	.	.	A	G	C	T	G	A
L. gasseri		.	-	A	.	.	A	T	.	.	.	.	.	.	.	.	.	.	C	T	A	G
L. iners		.	-	A	.	.	A	T	.	.	.	.	.	.	.	.	.	A	G	T	.	G
L. vaginalis		.	A	A	.	.	A	T	.	.	.	.	G	.	.	.	.	G	A	A	A	A

Table 3

Alignment of the 16S rRNA gene primers of A. vaginae with the sequences of the described Atopobium species

Forward primer (position 1006–1025)	5'
A. vaginae		G	G	T	G	A	A	G	C	A	G	T	G	G	A	A	A	C	A	C	T
A. fossor		.	.	.	.	.	.	.	.	G	.	C	.	.	.	.	.	.	G	T	C
A. minutum		.	.	.	.	.	.	.	.	G	.	C	.	.	.	.	.	.	G	T	C
A. parvulum		.	.	.	.	.	.	.	.	G	.	C	.	.	.	.	.	.	G	T	C
A. rimae		.	.	.	.	.	.	.	.	G	.	C	.	.	.	.	.	.	G	T	C
Reverse primer (position 1282–1265)	5'																				3'
A. vaginae		A	T	T	C	G	C	T	T	C	T	G	C	T	C	G	C	G	C	A
A. fossor		.	.	.	G	.	.	.	.	A	C	T	T	.	.	.	.	A	A	G
A. minutum		.	.	.	G	.	.	.	.	A	C	T	T	.	.	.	.	A	A	G
A. parvulum		.	.	.	.	.	.	.	C	A	C	C	.	.	.	.	.	.	G	G
A. rimae		.	.	.	.	.	.	.	C	G	C	C	.	.	T	.	.	.	G	G

Table 4

Overview of the primer sequences and PCR conditions as used in this study

Specificity	Name	Primer sequence (5'-3')	16S rDNA position^a (5'-3')	Cycling conditions	Reference
A. vaginae	ATOVAGRT3Fw	GGTGAAGCAGTGGAAACACT	1006–1025	10' 95°C, (15" 95°C, 20" 62°C, 40" 72°C) × 40	This study
	ATOVAGRT3Rev	ATTCGCTTCTGCTCGCGCA	1282–1265
G. vaginalis	F-GV1	TTACTGGTGTATCACTGTAAGG	16S-23S spacer	10' 95°C, (45" 94°C, 45" 55°C, 45" 72°C) × 50	[27]
	R-GV3	CCGTCACAGGCTGAACAGT	16S-23S spacer
L. crispatus	LcrisF	AGCGAGCGGAACTAACAGATTTAC	65–89	10' 95°C, (15" 95°C, 1' 60°C) × 40	[26]
	LcrisR	AGCTGATCATGCGATCTGCTT	205–185
L. gasseri	LactoF	TGGAAACAGRTGCTAATACCG	157–177	10' 95°C, (15" 95°C, 1' 60°C) × 40	[26]
	LgassR	CAGTTACTACCTCTATCTTTCTTCACTAC	470–442
L. iners	InersFw	GTCTGCCTTGAAGATCGG	70–85	10' 95°C, (1' 95°C, 1' 55°C, 1' 65°C) × 35	This study
	InersRev	ACAGTTGATAGGCATCATC	228–210
L. jensenii	LABJENTR2Fw	CCTTAAGTCTGGGATACCATT	117–137	10' 95°C, (15" 95°C, 10" 54°C, 30" 72°C) × 40	This study
	LABJENRT2Rev	ACGCCGCCTTTTAAACTTCTT	207–187

^aRelative to the position in the Escherichia coli 16S rDNA sequence.

Using Qiagen extracted DNA from pure cultures; the detection limit for A. vaginae is 1.3 pg/ml, for G. vaginalis 43.2 pg/ml, for L. crispatus 4.7 pg/ml, for L. gasseri 10.7 pg/ml, for L. iners 6.4 pg/ml and for L. jensenii 15.0 pg/ml.

Qualitative results

Table 5 presents the overall presence of the six species studied in the different grades of vaginal microflora. L. crispatus was found in all but 5 samples (93%) and was the most frequent Lactobacillus species detected. L. jensenii was found in 33 samples (46%) but especially in grade Iab where it was present in 8 of 10 samples (80%).

Table 5

Percentage of samples of each grade for which the tested species were detected

	Grade Ia	Grade Iab	Grade Ib	Grade I	Grade I-like	Grade II	Grade III	Grade IV	Total (%)
Number of samples	8	10	13	31	10	11	12	7	100
A. vaginae	38	20	15	23	30	18	83	14	32
G. vaginalis	88	50	61.5	65	70	63	100	29	68
L. crispatus	100	100	100	100	80	82	92	100	93
L. gasseri	88	90	85	87	60	100	33	43	72
L. iners	50	90	92	81	70	27	100	86	75
L. jensenii	13	80	46	48	60	55	50	0	47

Forty-eight samples (68%) were positive for G. vaginalis and 20/48 (42%) of these were also positive for A. vaginae. Only three samples were positive for A. vaginae but negative for G. vaginalis. All grade III samples were positive for G. vaginalis and 10/13 (83%) were also positive for A. vaginae.

L. gasseri was detected in 52/71 samples (73%) and 27/31 (87%) were grade I, 7/10 (70%) grade I-like, 11/11 (100%) grade II, 4/12 (33%) grade III and 3/7 (43%) grade IV.

L. iners was detected in 53/71 samples (75%) from which 25/31 (81%) were grade I, 7/10 (70%) grade I-like, 3/11 (27%) grade II, 12/12 (100%) grade III and 6/7 (86%) grade IV.

Quantitative results

Figure 2 and Table 6 give an overview of the results obtained with real-time PCR for four vaginal Lactobacillus species and for Gardnerella vaginalis and Atopobium vaginae.

Table 6

Quantitative determination of the six species in the different grades expressed as Median log₁₀ cells/ml (Interquartile Range)

	Grade I	Grade I-like	Grade II	Grade III	Grade IV
A. vaginae	0 (0 – 0)	0 (0 – 4.7)	0 (0 – 0)	9.0 (4.4 – 9.7)	0 (0 – 0)
G. vaginalis	5.1 (0 – 6.0)	5.4 (0 – 5.9)	4.7 (0 – 8.8)	9.2 (8.8 – 10.7)	0 (0 – 4.9)
L. crispatus	8.8 (5.6 – 9.5)	5.5 (2.8 – 6.2)	4.2 (3.6 – 5.1)	5.2 (4.3 – 5.6)	5.1 (4.7 – 5.9)
L. gasseri	6.6 (5.6 – 7.9)	6.4 (0 – 8.3)	8.7 (7.4 – 9.3)	0 (0 – 5.3)	0 (0 – 9.2)
L. iners	6.5 (3.7 – 8.6)	4.3 (3.9 – 4.5)	0 (0 – 3.8)	8.3 (5.6 – 8.7)	4.3 (3.9 – 4.5)
L. jensenii	4.0 (0 – 6.0)	4.3 (0 – 6.3)	4.3 (0 – 7.9)	2.1 (0 – 5.2)	0 (0 – 0)

Figure 2
**Overview of the results obtained with real-time PCR for** L. crispatus , L. jensenii , L. gasseri , L. iners , G. vaginalis **and** A. vaginae. x-axis: each bar represents a different sample. y-axis: logarithmic scale of cells/ml. Spaces in between horizontal lines represent log₁₀ 0.5 differences. Detection limits are 3.5 for *L. crispatus*, 4.0 for *L. jensenii*, 4.5 for *L. gasseri*, 3.5 for *L. iners*, 4.5 for *G. vaginalis* and 3.5 for *A. vaginae*. Data sorted per grade according to decreasing concentration of *L. crispatus*.

The median log₁₀ cells/ml were expressed as per 1 ml elution buffer.

We found a significantly higher level of L. crispatus in grade I (log₁₀ Median Concentration (MC) = 8.8 cells/ml) compared to the other grades, i.e. II: 4.2, p < 0.0001, III: 5.2, p = 0.002, IV: 5.1, p = 0.004 and I-like: 5.5, p = 0.014. L. crispatus was also present in significantly higher amounts in grade III compared to grade II (p = 0.023).

L. crispatus was present in high levels (i.e. at least log₁₀ 8.5 cells/ml) in all 8 grade Ia samples (log₁₀ MC = 9.0 cells/ml), in most (i.e. 6/10) grade Iab samples (log₁₀ MC = 8.9 cells/ml), but only in 3/12 grade Ib samples (log₁₀ MC = 5.6 cells/ml).

L. jensenii was found in all grades but showed higher concentration in grade Iab (log₁₀ MC = 7.0 cells/ml) than in grade Ia (log₁₀ MC = 0 cells/ml, p = 0.024)

The level of L. gasseri in grade I (log₁₀ MC = 6.6 cells/ml) was significantly lower than in grade II (log₁₀ MC = 8.7 cells/ml, p < 0.01) and significantly higher than in grade III (log₁₀ MC = 0 cells/ml, p < 0.0001). The quantity of L. gasseri in grade II was significantly higher than in grade III (p < 0.0001) and than in grade IV (log₁₀ MC = 0 cells/ml, p < 0.05).

The level for L. iners did not differ either between grades I and III or between grades I and I-like. L. iners was present in grade II (log₁₀ MC = 0 cells/ml) in significantly lower amounts than in grade III (log₁₀ MC = 8.3 cells/ml, p < 0.0001), in grade I (log₁₀ MC = 6.5 cells/ml, p < 0.0001), in grade IV (log₁₀ MC = 4.3 cells/ml, p < 0.05) and in grade I-like (log₁₀ MC = 4.3 cells/ml, p < 0.05).

The concentrations of A. vaginae and G. vaginalis were significantly higher in grade III (respectively log₁₀ MC = 9.0 cells/ml and 9.2 cells/ml) than in grade I (respectively log₁₀ MC = 0 cells/ml and 5.1 cells/ml, p < 0.0001), grade II (respectively log₁₀ MC = 0 cells/ml and 4.7 cells/ml p < 0.005), grade IV (respectively log₁₀ MC = 0 cells/ml and 0 cells/ml, p < 0.005 and p < 0.0001) and grade I-like (respectively log₁₀ MC = 0 cells/ml and 5.4 cells/ml, p < 0.005 and p < 0.0001). Concentrations of G. vaginalis were also higher in grade I than in grade IV (p < 0.05).

Significant positive correlations were found in our data set between L. jensenii and L. gasseri (r = 0.244, p < 0.05), between G. vaginalis and L. iners (r = 0.351, p < 0.05) and between G. vaginalis and A. vaginae (r = 0.469, p < 0.0001). Negative correlations were found between L. gasseri and L. iners (r = -0.397, p = 0.001) and between A. vaginae and L. gasseri (r = -0.408, p < 0.0001).

Gram staining of L. iners and L. gasseri

Figure 3 represents the Gram stains of 6 strains of L. gasseri and 6 strains of L. iners. Gram stains of L. iners and L. gasseri showed that many of these strains displayed pleiomorphic cell morphology, i.e. different cell types could be observed within one microscopic field. Also, the cell morphologies of strains differed within the same species. Most strikingly, all L. iners strains had a relatively Gram-negative stain appearance and were mostly very short rods. By contrast, the L. gasseri were clearly Gram-positive in all cases. Some strains of L. gasseri formed streptobacillar chains, consisting of long to extra-long rods.

Figure 3
**Microscopic images (100 ×) of Gram stains of** L. iners **and** L. gasseri. A-F: *L. iners*; A: BVS11, B: FB04-04, C: FB06-01, D: FB17-07, E: FB94-05b and F: FB30-01AN; G-L: *L. gasseri*: FB02-02, H: FB33-01, I: FB34-01AN, J: FB89-3, K: FB103-2, L: PB88-T2-1.

MIC of L. gasseri and L. iners for clindamycin

The clindamycin MIC value for ten strains of L. iners and L. gasseri was determined using the agar dilution method. Eight of the ten L. iners had a MIC value of 0.125 μg/ml, one strain had a MIC value of 2 μg/ml and one strain of >8 μg/ml. For L. gasseri one strain had a MIC value of 0.5 μg/ml, two strains had MIC values of 2 μg/ml, six strains had MIC values of 4 μg/ml and for one strain the MIC was more than 8 μg/ml. In summary, 80% of L. iners isolates were inhibited by 0.125 μg of clindamycin/ml, with MIC₅₀ = 0.125 μg/ml, whereas 90% of the L. gasseri isolates was resistant to 1 μg of clindamycin/ml, with MIC₅₀ = 4 μg/ml.

Mutual inhibition of L. gasseri and L. iners

No inhibition zones were observed with the techniques we used.

Discussion

In this study we used real-time PCR to obtain a quantitative estimation of the presence of the four predominant Lactobacillus species known to occupy the vaginal econiche and of Atopobium vaginae and Gardnerella vaginalis.

Real-time PCR has been applied previously for the description of changes in the vaginal microflora. Zariffard et al. [27] and Sha et al. [28, 29] used real-time PCR on frozen cervicovaginal lavage samples to quantify the presence of Mycoplasma hominis, G. vaginalis and the combined presence of L. crispatus and L. jensenii, in comparison with the microscopic interpretation of the Gram stain according to the criteria of Nugent [22]. Bradshaw et al. [16] applied real-time PCR for A. vaginae for a follow-up study of recurrent BV before and after treatment with oral metronidazole. Ferris et al. [17] applied real-time PCR for A. vaginae to samples of six BV patients before and after treatment with a topical metronidazole gel. Thus far, only one group (Byun et al. [26]), studying advanced dental caries, used real-time PCR to quantify the presence of specific Lactobacillus species.

Compared to microscopy and culture, molecular methods such as PCR may provide less observer-dependent and culture medium dependent information and a more direct and detailed view of the quantity of certain species in a sample. E.g., A. vaginae was only recently recognized as strongly linked to disturbed vaginal microflora because of its fastidious growth requirements in vitro. A possible additional advantage of PCR, compared to culture, is that it permits detection of dead or metabolically inactive bacteria, and as such it can be applied for the detection of bacteria in a dormant state, as is the case in biofilms, which occur also in BV as has been shown by means of FISH [12].

Besides culture-associated bias, difficulties with regard to the standardization of vaginal sampling make quantification of the vaginal microflora cumbersome and make bacterial counts reported in different publications difficult to compare. Some groups have attempted to standardize sampling by cervicovaginal lavage (CVL), whereby the volume of saline that is recovered from the vagina can be measured and used for calibration of the bacterial load/ml. Drawbacks are that CVL samples also from the cervix and does not represent a pure vaginal sample. Also it cannot be excluded that biofilm, that may be present in cases of BV, is recalcitrant with regard to dissolving in the saline that is used and is not sampled in the same manner as loosely associated microflora. In the condition of BV there may be more vaginal cell debris so it is feasible that there is more non-bacterial material present in the sample. In conclusion, vaginal sampling remains difficult to standardize. In this study we used unweighted vaginal swabs taken by the same gynecologist so there is no standardization for the volume of the sample, but standardization of the way samples are taken.

Besides sampling bias and culture bias also real-time PCR may be biased, because the conversion of the PCR positivity threshold value to a concentration of bacteria, depends on the manner the standard curve is calibrated. The standard curve, which is prepared by extracting DNA from a dense bacterial suspension and by serial tenfold dilution of this DNA extract, can be compared to i) the bacterial colony count, as determined by plating out tenfold serial dilutions of the initial suspension, or to ii) the number of bacterial genomes in the initial suspension, determined on the basis of measurement of the DNA-concentration present in the extract from the initial suspension. We found differences between calculation of number of genomes by measurement of DNA-concentration and determination of number of cells by dilution culture from less to one log₁₀ unit (L. jensenii) to more than 3 log₁₀ units (L. crispatus) (data not presented). A possible explanation may be that species like L. jensenii are more easily cultured on blood plates than for example L. crispatus and therefore show a lower discrepancy between DNA-concentration and culture. In conclusion, when preparation of the standard curve in this study had been based on cultured cells, L. jensenii would have been overestimated relative to the other species.

L. crispatus and L. jensenii

L. crispatus can be found in samples of all grades but the log₁₀ median concentration/ml (MC) of this species is much higher in grade I (8.8) compared to grades II (4.2) and III (5.2). Although the difference between the log₁₀ quantity of L. crispatus in grade Ia and grade Ib is not significantly different (p = 0.096), possibly because of the low sample size, a different profile is observed for these grades (Figure 2 and 3).

L. crispatus is present in high inoculum (i.e. at least) in all 8 grade Ia samples (log₁₀ MC 9.0), in most (i.e. 6/10) grade Iab samples (log₁₀ MC 8.9), but only in 3/12 grade Ib samples (log₁₀ MC = 5.6). Our study confirms that a grade Ia microflora is characterized by high concentrations of L. crispatus, whereas grades Iab and Ib consist of a more diverse microflora, with different Lactobacillus species present in comparable amounts.

Also, in grade Ib, high concentrations of L. crispatus can be found but on Gram stain especially long and small Lactobacillus cell types, which were suggested to be more typical for L. gasseri [24], are observed.

Based on cloning of the 16S rDNA library from the indigenous microbiota of three women with normal vaginal microflora, Verhelst et al. [14] found an almost pure population of L. jensenii in one of them and concluded that this species was associated with a normal vaginal microflora, but in this study (71 swabs) we can not correlate L. jensenii with either normal or disturbed vaginal microflora since it is present sporadically in samples of all grades, and in both high and low numbers. Its presence in 8/10 grade Iab samples, compared to 1/8 grade Ia samples is striking (p = 0.024).

G. vaginalis and A. vaginae

A positive correlation between G. vaginalis and A. vaginae could be established (p < 0.0001). G. vaginalis can be found in all grades but in much higher concentration in a disturbed vaginal microflora. Delaney et al. [30] performed a comparative study in which they quantified G. vaginalis, Lactobacillus spp., Prevotella spp. and Peptostreptococcus spp. in vaginal swabs by means of culture. The mean log₁₀ number of G. vaginalis in BV was determined to be 9.64 cfu/g, which may compare well to the value we obtained, i.e. 9.2 cells/ml in grade III.

A. vaginae is found less frequently than G. vaginalis in non-grade III samples, but in high concentrations in 10 of the 12 grade III samples, confirming that the presence of A. vaginae seems to be a diagnostically more valuable marker for BV than the presence of G. vaginalis, as suggested by Verhelst et al. [14] and confirmed by several other studies [31–33]. A recent study using T-RFLP for the characterization of normal (n = 20) and BV (n = 50) microflora found that the terminal restriction fragment (TRF) with the length to that corresponding of A. vaginae was present in the vagina of 48 of the 50 women with BV (grade II and III lumped together) and absent from all 20 women with normal microflora [32]. Bradshaw et al. [16] and Ferris et al. [17] monitored the changes in the concentration of A. vaginae before and after treatment with metronidazole and both found that very high vaginal concentrations of A. vaginae were predictive for patients for whom treatment failed partially or completely, although Bradshaw et al. [16] found a significant reduction of A. vaginae after metronidazole treatment. This might be due to a lower susceptibility of some strains of A. vaginae for metronidazole [34] but a more plausible explanation might be the existence of biofilm as shown by Swidsinski et al. [12], and in which G. vaginalis was shown to be associated with A. vaginae.

L. gasseri and L. iners

Overall L. gasseri and L. iners are abundantly present in most grades. Strikingly, L. gasseri is virtually absent in grade III whereas L. iners is virtually absent in grades Ia and II.

In our study we found a high concentration of L. iners to be clearly associated with low concentrations of L. gasseri, which is more prevalent in normal (grade Ia, grade Ib, grade Iab) and mildly disturbed flora (grade II). This was confirmed by Spearman rank testing, which showed that L. gasseri and L. iners are significantly negatively correlated to each other in grades II and III (r = -0.793, p < 0.0001), but also when all samples are considered together (r = -0.397, p = 0.001).

It can be noted that even the single grade III sample with a high concentration of L. gasseri was also one of the two grade III samples with low concentration of L. iners. In addition, we found a positive correlation between G. vaginalis and L. iners. The distribution frequencies over the different grades of L. iners and G. vaginalis are quite similar, i.e. present in most grades but predominantly in grade III, but different from A. vaginae, i.e. present almost exclusively in grade III, which may explain why L. iners does not correlate with A. vaginae. This distribution of L. iners was also observed in the T-RFLP study of Thies et al. [32], with 32 out of 50 BV samples and 11 out of 20 normal microflora samples containing the L. iners TRF. The L. gasseri group TRF was observed only twice, in women with normal microflora. Unfortunately, these authors did not distinguish between grade II and III.

According to some research groups [35], L. iners is the most abundant vaginal Lactobacillus species, not only in black African women (64% of 241 healthy premenopausal Nigerian women) but also in white women from Sweden, the US and Canada and is considered as even more typical for normal vaginal microflora than L. crispatus. Although L. iners was present in high numbers in grades Iab and Ib, we found L. crispatus and L. gasseri to be more abundant in grade Ia. Ferris et al. [17] concluded that L. iners is a more transitional species, present in recently cured patients. They reported the predominance of L. iners in 5 patients with BV after metronidazole treatment, whereas for the sixth patient, the only one with a complete treatment failure, L. iners was present but not predominant. These results were confirmed by Jakobsson and Forsum [36].

Interestingly, it has been observed by the group of Taylor-Robinson that grade II microflora responds poorly to clindamycin treatment whereas most subjects with grade III microflora readily reverted to grade I [37, 38] and also that women with clindamycin treated grade III microflora had a better pregnancy outcome than women with clindamycin treated grade II microflora [37]. In agreement, the predominance of clindamycin susceptible L. iners in grade III might explain the observations of Taylor-Robinson et al. [38].

Finally, in case grade II would be an intermediate stage in between transition from grade I to grade III, one would expect to see an increase in L. iners and a decrease in L. gasseri, since the former is present in high numbers in grade III and the latter almost absent, but we observe exactly the opposite, i.e. nearly complete absence of L. iners and high numbers of L. gasseri in grade II.

In order to establish whether this could be related to the differential presence of L. gasseri and L. iners in these grades, with L. gasseri predominant in grade II, we determined the MIC for clindamycin for 10 strains of each. We found that 8 out of 10 L. iners strains were inhibited by less than 0.25 μg/ml, whereas 9 out of 10 L. gasseri strains had a MIC value of 2 or more μg clindamycin/ml. Although L. gasseri cannot be considered definitely as the causative micro-organism responsible for the adverse pregnancy outcome that has been associated with grade II, our data indicate that it can be considered as contributing to the poor response to clindamycin treatment.

To test the hypothesis that L. gasseri and L. iners are mutually exclusive, e.g. by the production of bacteriocins, we carried out inhibition tests between both species. However, with the method we used we could not observe mutual inhibition between both species.

With the use of molecular techniques it becomes clear that the definition for bacterial vaginosis in which it is claimed that the lactobacilli are replaced by anaerobic bacteria is not quite correct. Our data indicate that rather L. crispatus, L. gasseri and L. jensenii present in a healthy vaginal microflora and grade II microflora are replaced largely by L. iners in grade III vaginal microflora. Accordingly, the qualitative culture study by Delaney & Onderdonk [30] found a weak negative correlation between Nugent score and numbers of all lactobacilli, meaning that the number of lactobacillar cells did not decrease with high Nugent score, i.e. disturbed microflora. On the other hand, Zariffard et al. [27] and Sha et al. [28, 29] who quantified lactobacilli in cervicovaginal lavage samples, using a real-time PCR format which picked up only L. crispatus and L. jensenii, found a decline in the number of lactobacilli in BV. The discrepancy may be explained because we take also L. iners and L. gasseri into account.

To further resolve these discrepancies we carried out Gram staining of several strains of each L. gasseri and L. iners. It is of importance to note that L. iners has not only long escaped from our attention due to its inability to grow on MRS agar, but also hides as a Lactobacillus from Gram stains, because it stains Gram-negative and its cell morphology is rather coccobacillar than bacillar. Since it is the predominant Lactobacillus species in BV microflora – even present in high numbers – this has led to the false assumption that the BV microflora is devoid of lactobacilli.

The very long lactobacillar cells observed for some of the L. gasseri isolates remind of earlier observations. Pahlson & Larsson [39] reported the occurrence of very long fusiform lactobacilli in 7.4% of the vagina of 981 women studied. Horowitz et al. [40] reported the occurrence of 'vaginal lactobacillosis', a pathological condition characterized by the presence of extremely long lactobacilli (up to 60 μm).

Grade I-like was described only recently by Verhelst et al. [24] as a grade that, on Gram stain, resembles grade I because of the Gram positive rods, but with the use of molecular methods it was shown that these rods were Bifidobacterium spp. instead of Lactobacillus spp.

Again this study confirms the separate nature of grade I-like vaginal microflora. A significantly lower concentration of L. crispatus (log₁₀ MC = 5.5 cells/ml) is present compared to grade I (log₁₀ MC = 8.8 cells/ml, p = 0.014) and much lower concentrations of G. vaginalis (log₁₀ MC = 4.0 cells/ml, p < 0.0001) and A. vaginae (log₁₀ MC = 1.6 cells/ml, p = 0.003) are present in grade I-like microflora compared to grade III (respectively log₁₀ MC = 9.2 cells/ml and log₁₀ MC = 9.0 cells/ml).

Conclusion

We report a strong negative association between L. iners and L. gasseri, whereas L. gasseri is predominant in grade II and L. iners in grade III. It has been mentioned by others [5] that a grade II microflora is not necessarily intermediate between grade I and III.

L. iners and L. gasseri do not inhibit each other by production of bacteriocins, according to the technique we used. In addition we found L. iners to be very sensitive for clindamycin (MIC₅₀ = 0.125 μg/ml) compared to the higher MIC value for L. gasseri (MIC₅₀ = 4 μg/ml). Comparison of these results with findings of other research groups is very difficult because L. iners has long been overlooked in culture and Gram stain. The unexpected Gram negative pleiomorphic cell shape of L. iners, as established in this study, and its inability to grow on MRS agar made the estimation of the occurrence of this species almost impossible until the recent development of molecular techniques.

Methods

Strains and culture conditions

The specificity of the primer set for Lactobacillus iners was tested using the following strains: L. iners (CCUG 28746^T), L. brevis (LB4), L. delbrueckii (LB31), L. crispatus (ATCC 33199^T), L. casei (ATCC 393^T), L. fermentum (ATCC 23271, ATCC 11739^T, SAV1, SAV 3, SAV5), L. gasseri (ATCC 33323^T), L. jensenii (ATCC 25258^T), L. johnsonii (DSM 20553), L. plantarum (ATCC 8014, ATCC 10012, ATCC 14917^T), L. reuteri (ATCC 23272^T, RC-14), L. rhamnosus (ATCC 7469^T, GR-1, GG) and L. salivarius (SAV6).

The specificity of the primer set for Lactobacillus jensenii was tested using the following strains:L. acidophilus (LMG 11430), L. animalis (LMG 9843^T), L. bifermentans (LMG 11431), L. brevis (LMG 7761), L. casei (FB86-16), L. coleohominis (PB2003/024-T1-1a), L. crispatus (LMG 9479^T), L. curvatus (0606 93811c), L. delbrueckii (LMG 6412^T), L. fermentum (LMG 6902^T), L. gasseri (LMG 9203^T), L. helveticus (LBP152), L. iners (BVS11, PB2003/044-T1-1, PB2003/53-T1-1), L. intestinalis (LMG 14196^T), L. jensenii (PB2003/204-T1-1, FB65-6, FB122-BP-1, FB146-BA-5, FB154-CAN-2), L. johnsonii (LBP151), L. plantarum (LMG 9212), L. reuteri (LMG 9213T), L. rhamnosus (LMG 8153, LMG18243), L. salivarius (LMG 9477^T) and L. vaginalis (LMG 12891^T).

The specificity of the primer set for Gardnerella vaginalis was tested using the following strains: Bifidobacterium infantis (PB2003/126-T1-3), B. breve (PB2003/108-T1-1) and B. bifidum (PB2003/99-T1-2).

The specificity of the primer set for Atopobium vaginae was tested using the following strains: A. minutum (CCUG 31167), A. parvulum (CCUG 32760), A. rimae (CCUG 31168) and A. vaginae (CCUG 38953^T, CCUG 42099, CCUG 44116, CCUG 44125, PB2003/189-T1-4). All strains were cultured on Trypticase soy agar with 5% sheep blood (Becton Dickinson, Erembodegem, Belgium) in anaerobic conditions (Gaspak, Becton Dickinson) for 72 hours at 37°C.

Samples

A total of 142 swabs (Copan, Brescia, Italy) were collected by sampling 60 women of childbearing age (32 pregnant women, 28 non-pregnant women). Sampling was carried out by insertion of two sterile cotton swabs into the vaginal vault, after placement of a non-lubricated speculum. The swabs were rotated against the vaginal wall at the mid-portion of the vault and were carefully removed to prevent contamination with microflora of the vulva and introitus. The first swab was used to prepare a smear on a glass slide for the purpose of grading as described by Verhelst et al. [14]. The second swab was returned to a sterile tube for the purpose of DNA extraction (dry swab). Both swabs were sent to the microbiology laboratory and were processed within 4 hours.

The study protocol was approved by the ethical committee of the Ghent University Hospital and individual written informed consent was obtained.

DNA extraction of bacteria and samples

DNA was extracted from cultured bacteria by simple alkaline lysis. One colony was suspended in 20 μl of lysis buffer (0.25% SDS, 0.05 N NaCl and 95 ml sterile distilled water) and heated for 15 minutes at 95°C. After briefly centrifugating, 180 μl of HPCL-water was added and this was centrifuged again for 5 minutes at 16300 g. Concentrations of DNA-extracts ranged between 2.1 and 87.5 ng/μl.

For dry vaginal swabs, the QIAamp DNA mini kit (Qiagen, Hilden, Germany) was used according to the manufacturer's recommendations, with minor modifications. The dry swab specimen from each patient was swirled for 15 s in 400 μl of lysis buffer (20 mM Tris-HCl, pH 8.0; 2 mM EDTA; 1.2% Triton). Fifty units of mutanolysin (25 U/μl) (Sigma, Bornem, Belgium) were added and the samples were incubated for 30 min at 37°C. After the addition of 20 μl Proteinase K (20 mg/ml) and 200 μl AL buffer (Qiagen), samples were incubated for 30 min at 56°C. Next, 200 μl of ethanol was added and DNA was purified by adding the lysate to the Qiagen columns as described by the manufacturer. Finally, the total bacterial DNA was eluted with 100 μl of AE buffer (Qiagen). DNA extracts were aliquoted and stored at -20°C.

Primers

PCR primer sets targeting L. iners, L. jensenii and A. vaginae were designed by aligning the sequences of the 16S rRNA gene of different strains of both species by CLUSTALW [41]. Specificity of the primer sets (Eurogentec, Seraing, Belgium) was analyzed by using the BLAST algorithm [42]. Primer sequences for L. jensenii and L. iners alignment to the most common vaginal lactobacilli are shown in Table 1 and Table 2. Primer sequences for A. vaginae and alignment to other members of the Atopobium group are shown in Table 3. Position of the primers on the 16S rRNA-gene is shown on Figure 1. Optimal annealing temperature of each primer set was established by gradient PCR and analysis on an agarose gel. In addition, already described primers for L. crispatus and L. gasseri [26] and G. vaginalis [27] were used. Primer sequences and cycling conditions are summarized in Table 4. Primer concentrations were 100 nM each except for the assays for G. vaginalis and L. iners for which the primer concentrations were 200 nM.

Construction of the standard curves for real-time PCR

To construct standard curves for the real-time PCR's, A. vag inae (CCUG 38953^T), L. crispatus (PB2003/125-T1-1), L. gasseri (FB102-1) and L. jensenii (PB2003/204-T1-1) were cultured on TSA + 5% sheep blood (Becton Dickinson) and G. vaginalis (LMG 7832^T) and L. iners (BVS11) were cultured on CNA agar (Becton Dickinson) + 5% human blood. A suspension was made in MRS Broth (Oxoid, Drongen, Belgium) and DNA was extracted. The DNA concentration of this stock was determined ten times by using the Nanodrop ND-1000 (Nanodrop Technologies, Wilmington, USA) and the mean value was used for further calculations. For each strain a tenfold dilution series was prepared by dilution of the DNA stock in HPLC grade water. Dilutions were aliquoted and stored frozen at -20°C.

Real-time PCR

The qPCR Core Kit for SYBR Green I (Eurogentec) was applied and analysis was performed on the ABI 7300 real-time PCR system (Applied Biosystems, Foster City, CA).

Reactions were done in PCR mixtures containing 2.5 μl of DNA extract, 2.5 μl of 10 × Reaction Buffer, 3.5 mM MgCl₂, 0.2 mM dNTP mixture, 0.625 U HotGoldStar Taq polymerase, 0.75 μl SYBR^® Green I, diluted 10-fold in DMSO and the appropriate primer concentration, adjusted with HPLC grade water to 25 μl. Primer concentrations are summarized in Table 4. Each run included a standard curve and each sample was run in triplicate. In case the result was not in the range of the standard curve, the samples were diluted tenfold and analyzed in triplicate again. The median log₁₀ cells/ml were expressed as per 1 ml elution buffer.

Agar dilution method

Clindamycin (Sigma, Bornem, Belgium) minimal inhibitory concentrations (MIC) were determined for 10 strains of L. gasseri ( FB02-02, FB13-01, FB29-6, FB34-01AN, FB86-6, FB89-3, FB102-1b, FB103-2, PB88-T2-1 and PB327-1) and 10 strains of L. iners (BVS11, FB04-04, FB05-01, FB06-01, FB07-01, FB17-07, FB30-01AN, FB77-03, FB94-05b and FB123-CNA-4) using the agar dilution method on Trypticase Soy Agar (Becton Dickinson) + 5% human blood and incubation anaerobically during 72 hours at 37°C in the Anaerobic Workstation BugBoxPlus (LED Techno, Heusden-Zolder, Belgium). Concentrations of 8, 4, 2, 1, 0.5, 0.250, 0.125 and 0.0625 μg/ml, were tested for each strain in triplicate.

Mutual inhibition test

The same strains used for MIC-determination were grown in Trypticase Soy Broth (Becton Dickinson) + 5% human blood for 72 hours at 37°C in the anaerobic workstation BugBoxPlus (LED Techno, Heusden-Zolder, Belgium). Supernatant of the liquid cultures and of the negative control were sterilized trough a 0.22 μm filter (Spin-X Centrifuge Tube Filter, Costar, Corning, NY14831). Plates were inoculated with a swab to obtain confluent growth. Volumes of 20 μl of the filter sterilized supernatants were dropped onto the inoculated plates, followed by anaerobic incubation at 37°C for 72 hours, whereafter inhibition zones were recorded.

Data analysis

For the calculation of number of cells in each dilution, genome size and % G+C of the bacterial species was taken into account. The genome size of G. vaginalis (ATCC 14019, ATCC 14018, GVP 007 and GVP 004) has been approximated to 1.7 Mb [43] and % G+C was 43 [44]. For L. gasseri data described for strain ATCC 33323 (genome size: 1.9 Mb, 35.3% G+C) [45] were used. Also for A. vaginae strain CCUG 38953^T (44% G+C) [46], L. crispatus strain ATCC 33820^T (35% G+C) [47], L. iners strain CCUG 28746^T (34.4% G+C) [20] and L. jensenii strain ATCC 25258^T (36.1% G+C) [48] a genome size of 1.9 Mb was assumed.

Statistical analysis

Data were analyzed under the non-parametric assumption, taking into consideration the log₁₀ [count] distributions of species under study did not approximate the normal distribution. For any given category (grades I-IV) the distribution of concentrations (log₁₀ cells/ml) of each species was expressed as the median count and the accompanying interquartile range (IQR). Between group comparisons of distributions were performed with the Mann-Whitney U-test for two groups and with the Kruskal Wallis test for multiple groups. Correlations between the different species were determined by the Spearman (rank) test and reported as Spearman's rho value (r). All analyses were performed using SPSS v15 software (Chicago, Illinois).

Declarations

Acknowledgements

Ellen De Backer is indebted for a PhD Research funded by the Institute for the Promotion of Innovation through Science and Technology in Flanders (IWT-Vlaanderen).

Authors’ Affiliations

(1)

Department of Clinical Chemistry, Microbiology & Immunology, Ghent University Hospital, UGent, Belgium

(2)

Department of Obstetrics & Gynaecology, Ghent University Hospital, UGent, Belgium

(3)

Department of Microbiology and Immunology, University of Otago, Dunedin, New Zealand

(4)

BLIS Technologies Ltd., Centre for Innovation, University of Otago, Dunedin, New Zealand

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This article is published under license to BioMed Central Ltd. This is an Open Access article distributed under the terms of the Creative Commons Attribution License (http://creativecommons.org/licenses/by/2.0), which permits unrestricted use, distribution, and reproduction in any medium, provided the original work is properly cited.

Quantitative determination by real-time PCR of four vaginal Lactobacillus species, Gardnerella vaginalis and Atopobium vaginae indicates an inverse relationship between L. gasseri and L. iners

Abstract

Background

Results

Conclusion

Keywords

Background

Results

Grading of vaginal microflora

Primer development and real-time PCR format

Qualitative results

Quantitative results

Gram staining of L. iners and L. gasseri

MIC of L. gasseri and L. iners for clindamycin

Mutual inhibition of L. gasseri and L. iners

Discussion

L. crispatus and L. jensenii

G. vaginalis and A. vaginae

L. gasseri and L. iners

Conclusion

Methods

Strains and culture conditions

Samples

DNA extraction of bacteria and samples

Primers

Construction of the standard curves for real-time PCR

Real-time PCR

Agar dilution method

Mutual inhibition test

Data analysis

Statistical analysis

Declarations

Acknowledgements

Authors’ Affiliations

References

Copyright

BMC Microbiology

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