Listeria monocytogenes Wall Teichoic Acid Glycosylation Promotes Surface Anchoring of Virulence Factors, Resistance to Antimicrobial Peptides, and Decreased Susceptibility to Antibiotics

Abstract

The cell wall of Listeria monocytogenes (Lm), a major intracellular foodborne bacterial pathogen, comprises a thick peptidoglycan layer that serves as a scaffold for glycopolymers such as wall teichoic acids (WTAs). WTAs contain non-essential sugar substituents whose absence prevents bacteriophage binding and impacts antigenicity, sensitivity to antimicrobials, and virulence. Here, we demonstrated, for the first time, the triple function of Lm WTA glycosylations in the following: (1) supporting the correct anchoring of major Lm virulence factors at the bacterial surface, namely Ami and InlB; (2) promoting Lm resistance to antimicrobial peptides (AMPs); and (3) decreasing Lm sensitivity to some antibiotics. We showed that while the decoration of WTAs by rhamnose in Lm serovar 1/2a and by galactose in serovar 4b are important for the surface anchoring of Ami and InlB, N-acetylglucosamine in serovar 1/2a and glucose in serovar 4b are dispensable for the surface association of InlB or InlB/Ami. We found that the absence of a single glycosylation only had a slight impact on the sensibility of Lm to AMPs and antibiotics, however the concomitant deficiency of both glycosylations (rhamnose and N-acetylglucosamine in serovar 1/2a, and galactose and glucose in serovar 4b) significantly impaired the Lm capacity to overcome the action of antimicrobials. We propose WTA glycosylation as a broad mechanism used by Lm, not only to properly anchor surface virulence factors, but also to resist AMPs and antibiotics. WTA glycosyltransferases thus emerge as promising drug targets to attenuate the virulence of bacterial pathogens, while increasing their susceptibility to host immune defenses and potentiating the action of antibiotics.

1. Introduction

Listeria monocytogenes (Lm) is a major intracellular foodborne bacterial pathogen that causes listeriosis, a human systemic infection [1]. Among zoonotic diseases under European Union (EU)-surveillance, listeriosis is the most severe [2]. Lm has the capacity to colonize various niches, from inert and organic matrices to the intestinal lumen where it competes with resident microbiota, translocates across the epithelium, multiplies in phagocytic and non-phagocytic cells, and disseminates via the blood [1,3].

In Gram-positive bacteria, the peptidoglycan (PGN) is densely decorated with glycopolymers such as lipoteichoic acids (LTAs), anchored to the head groups of membrane lipids by a diacylglycerol, and wall teichoic acids (WTAs), which are covalently attached to PGN via phosphodiester linkage [4,5]. WTAs are the most abundant PGN-linked polymers in Gram-positive pathogens such as Lm and Staphylococcus aureus. They play key functional roles in bacterial physiology, including cation binding, osmotic and heat tolerance, regulation of autolytic activity, cell-shape determination, and phage-binding [6]. Furthermore, WTAs have important roles in Gram-positive bacteria pathogenicity, namely by coordinating the mechanisms required for host infection and colonization, and conferring resistance to antimicrobial peptides (AMPs) and decreased susceptibility to antibiotics [6].

In Lm, WTAs are composed of repeated ribitol-phosphate (RboP) subunits, whose hydroxyl groups can be substituted by diverse monosaccharides [4,7]. Specific substitutions are characteristic of specific Lm serovars (Sv), namely: l-rhamnose (Rha) and N-acetylglucosamine (GlcNAc) in Sv1/2 and d-glucose (Glu), and d-galactose (Gal) in Sv4 [8]. Sv-specific phage resistance and virulence attenuation have been attributed to alterations in WTA-glycosylation (WTA-gly) [9,10,11,12,13,14]. Phage predation depends on specific WTA sugar residues and represents a driving force for Lm evolution [15]. Importantly, the majority of listeriosis outbreaks have been associated with Sv1/2 and Sv4b [16].

It was previously demonstrated that Lm strain EGDe (Sv1/2) WTA decorated with Rha (WTA-Rha) requires both RmlACBD biosynthetic enzymes and the rhamnosyltransferase RmlT, and confers resistance to the action of AMPs [17]. Importantly, we proved that the increased Lm susceptibility to AMPs, in the absence of WTA-Rha, is as a result of an increased cell wall permeability, which results in a faster plasma membrane disruption, with lethal consequences for bacteria. WTA-Rha has been clearly shown to be required for Lm virulence, but not for growth in an AMP-defective host [17].

The cell wall of Gram-positive bacteria is also the docking site for proteins covalently bound to PGN or noncovalently retained via the interaction with cell wall components [4]. Numerous Lm virulence factors are cell wall-associated proteins [3], including InlB and Ami [18,19]. While the cell wall retention of these proteins was previously shown to be partially dependent on LTA and PGN [20,21], WTA-Rha was proven to be essential for their proper surface anchoring [22]. More recently, the loss of WTA-Gal in Sv4b has been shown to not only prevent phage adsorption, but also to lead to a complete loss of surface-associated InlB and virulence attenuation in vivo [23]. Importantly, glycosylated WTAs have been described as being required for decreased susceptibility to antibiotics in S. aureus [24].

Our aim here was to analyze if other WTA glycosylations could have an equivalent role on the surface association of virulence factors and resistance to antimicrobial peptides, and to demonstrate the role of WTA glycosylation in Listeria sensitivity to antibiotics.

2. Results

2.1. WTA-glycosylation Promotes Efficient Surface Association of Lm Virulence Factors

Previous studies have shown that WTA-Rha in Lm Sv1/2a is required for the surface anchoring of virulence factors, namely Ami and InlB [22]. Similarly, the absence of WTA-Gal in Sv4b causes the complete loss of surface-associated InlB [23]. Given that, besides Rha and Gal, Lm WTAs can be modified with GlcNAc or Glu moieties, we wondered whether the association of Ami and InlB to the bacterial surface could be broadly dependent on WTA glycosylation events.

We assessed the surface association and culture media secretion of Ami and InlB in Lm Sv1/2a WT, as well as in isogenic mutants deficient for WTA-Rha (ΔrmlT), WTA-GlcNAc (Δlmo1079) and for both glycosylations (Δlmo1079ΔrmlT) (Figure 1 and Figure S1A). We first confirmed that mutant and wild type (WT) strains grow with comparable rates in a brain heart infusion (BHI) medium at 37 °C, indicating that the absence of any of WTA glycosylation does not impair bacterial growth in pure culture (Figure 1A). The presence of Ami and InlB on the extracts of non-covalently associated surface proteins and on culture supernatants collected from exponential growth cultures was assessed by Western blot analysis. Ami, in its unprocessed (~100 kDa) and processed forms [19], was detected in extracts of surface associated proteins from WT and mutant strains (Figure 1B). As previously described for the WTA-Rha deficient strain (ΔrmlT) [22], the levels of surface associated Ami were also slightly reduced in the mutants lacking WTA-GlcNAc (Δlmo1079) or both Rha and GlcNAc (Δlmo1079ΔrmlT) as compared to the WT strain (Figure 1B). Strikingly, while Ami was undetectable in the secreted protein extracts from WT Sv1/2a, all of the Ami forms were strongly detected in the culture supernatants from mutants deficient in specific WTA-glycosylations (Figure 1B), demonstrating that both WTA-Rha and WTA-GlcNAc are necessary for full the retention of Ami in a bacterial surface, avoiding its release to the extracellular milieu. As previously reported [22], the WTA-Rha deficient mutant (ΔrmlT) show consistently reduced levels of surface-bound InlB and increased InlB amounts in the supernatant fraction compared with WT (Figure 1B). In contrast, the absence of WTA-GlcNAc did not interfere with the InlB surface association or secretion (Figure 1B).

We extended our experimental approach to the Lm Sv4b strain, in which WTAs are decorated with Glu and Gal. We used WT Sv4b as well as strains deficient in WTA-Gal (ΔgttA), WTA-Glu (ΔgltB), and both glycosylations (ΔgttAΔgltB). The growth rate of mutant strains was comparable to that of the WT in BHI at 37 °C (Figure 1C). Two forms of Ami were detected in the non-covalently associated surface protein extracts of the WT Sv4b strain, with none of these forms being secreted to the culture medium (Figure 1D). The surface association of the 85 kDa unprocessed Ami remained unchanged in the WTA-Gal (ΔgttA) and WTA-Glu (ΔgltB) mutants, as well as in the double mutant (ΔgttAΔgltB). However, in the strains lacking WTA-Gal (ΔgttA and ΔgttAΔgltB), the Ami processed form (75 kDa) was decreased in the surface extracts and strongly increased in the secreted extracts (Figure 1D), indicating that WTA glycosylation with Gal is essential for the surface association of the processed form of Ami. As previously reported [23], the absence of WTA-Gal (ΔgttA and ΔgttAΔgltB) induced an almost complete secretion of InlB (Figure 1D). However, in the absence of WTA-Glu (ΔgltB), both Ami and InlB display surface association/secretion patterns similar to the WT strain (Figure 1D).

Altogether, these results indicate that, depending of the serovar, specific WTA-glycosylations are crucial for the efficient surface association of Lm virulence factors, namely Ami and InlB.

2.2. WTA-glycosylation Promotes Lm Resistance to AMPs

In Lm Sv1/2a, WTA-Rha contributes to resistance against host AMPs [17]. Here, we analyzed whether other WTA glycosylations could also promote Lm resistance against AMPs. To evaluate the role of WTA-GlcNAc in Lm Sv1/2a resistance to AMPs, we assessed the in vitro survival of Lm Δlmo1079, as compared with the WT and ΔrmlT strains, in the presence of biologically active human LL-37 and its mouse homologue cathelicidin-related antimicrobial peptide (CRAMP; Figure 2 and Figure S1B). After two hours of incubation with AMPs, the surviving bacteria were quantified by colony-forming unit CFU counting (Figure 2A,C). Compared with the WT strain, the Δlmo1079 mutant displayed a slight increased susceptibility to CRAMP as the ΔrmlT strain (Figure 2A, upper left panel). Interestingly, the double mutant Δlmo1079ΔrmlT, lacking both Rha and GlcNAc, displayed a significant increased susceptibility to both CRAMP and LL-37 (Figure 2A, right panels), indicating that WTA-Rha and WTA-GlcNAc cooperate to confer Lm resistance to AMPs. To further corroborate these data, the growth of Lm WT, Δlmo1079 and Δlmo1079ΔrmlT strains, in the presence of CRAMP or LL-37 (10 μg/mL) was monitored over time through optical density measurement (Figure 2B). According to the survival data, we observed a slight but significant growth defect for the Δlmo1079 strain in the presence of CRAMP. In turn, the double Δlmo1079ΔrmlT mutant showed a significant growth defect in the presence of CRAMP or LL-37, confirming that both Rha and GlcNAc of the Lm WTAs are important to confer resistance to AMPs.

The role of Gal and Glu in the resistance of the Lm Sv4b strain against AMPs was also assessed. Similar to the Sv1/2a strain, incubation with CRAMP only induced a slight decrease in the survival levels of single mutants (ΔgttA and ΔgltB). LL-37 had no effect on the survival of ΔgttA and ΔgltB strains, as compared with WT (Figure 2C). However, the double mutant ΔgttAΔgltB, lacking both WTA-Glu and -Gal, displayed a dramatic increase in susceptibility to both CRAMP and LL-37 (Figure 2C).

In agreement, besides slight differences observed in the bacterial growth of single mutants in the presence of 10 μg/mL of AMPs, the double mutant exhibited clear growth defects in the presence of both AMPs, as compared with the WT strain (Figure 2D).

Altogether, these results demonstrate the role of different WTA glycosylations in the susceptibility to AMPs of diverse Lm serovars, and highlight the cooperative role of distinct glycosylations.

2.3. WTA-glycosylation Promotes Lm Decreased Susceptibility to Some Antibiotics

Then, we analyzed the potential role of WTA glycosylations in Lm susceptibility to antibiotics. We tested β-lactams (ampicillin and penicillin) and aminoglycoside (gentamicin), which are antibiotics commonly used in clinics for the treatment of human listeriosis [25].

Minimum inhibitory concentrations (MICs) were determined by the Epsilometer test (E-test) method. Lm Sv1/2a and Sv4b showed a similar susceptibility towards penicillin and gentamicin (Figure 3A). However, Lm Sv4b appeared slightly less susceptible to ampicillin.

In the Lm Sv1/2a strain, the absence of WTA-Rha induced a slight increase in bacterial susceptibility to gentamicin. Remarkably, the double mutant lacking both Rha and GlcNac (Δlmo1079ΔrmlT) showed an increased susceptibility to all of the antibiotics tested (Figure 3A). In the Sv4b strain, the simultaneous loss of Gal and Glu in WTAs (ΔgttAΔgltB strain) also increased antibiotic sensitivity (Figure 3B).

Altogether, these results indicate that WTA glycosylations confer a specific decreased susceptibility to antibiotics, depending on the type of glycosylation and on the antibiotics, revealing the important role of WTA glycosylations in Lm susceptibility to antibiotics.

3. Discussion

While killing/inhibiting the growth of sensitive strains, conventional antibiotics enable resistant bacteria to grow in a competitor-free environment, creating strong selection for resistance. Rather than to kill or halt bacterial growth, one attractive strategy to disarm pathogens is by directly targeting virulence and/or resistance mechanisms using drugs that do not directly harm their targets, and thus do not impose resistance selection. Another promising approach is sensitizing bacteria from already existing drugs. The idea is to develop compounds that do not directly kill bacteria, but selectively disarm them, giving antibiotics the chance to act. Importantly, “disarm—do not kill” approaches also overcome two major antibiotics shortfalls, namely: drug resistance development and the killing of commensal bacteria.

Here, we demonstrated that WTA glycosylation appears to be a broad mechanism used by Lm not only to anchor virulence factors at its surface, but also to overcome the action host AMPs and antibiotics. Further studies should evaluate the role of WTA glycosylation in other Lm serovars.

To efficiently infect its host, Lm makes use of a large array of virulence effectors that act at different steps of the infection cycle [3]. Lm virulence factors include bacterial surface proteins that are associated with the cell wall. Their extra-cytoplasmic localization allows these proteins to interact directly with host cell targets, and to induce the effects necessary for the establishment of infection. The association of two of these virulence factors, Ami and InlB, at the bacterial surface was previously shown to be dependent on WTA-Rha [22]. Here, we demonstrate WTA glycosylation as a broad mechanism modulating proper protein association to the bacterial surface in diverse Lm Sv. In addition to WTA glycosylations, surface localization also depends on the protein itself. Ami and InlB belong to a protein family whose association to the bacterial surface is promoted by Glycine-Tryptophan (GW) modules. GW modules are sufficient for their WTA-Rha dependent surface localization; however, this is not the case for all Lm proteins containing GW modules [22]. Very recently, WTA-Gal was shown to be required for the stable surface association of another important Lm virulence factor, ActA, whose surface localization is unrelated to GW modules. The absence of WTA-Gal induces ActA secretion, and a concomitant loss of ActA-mediated intracellular motility and virulence [26]. This is in agreement with the decreased actin tail formation observed in a Sv4b WTA-Gal deficient mutant [23]. Altogether, these results point to a broad role of WTA glycosylations in the surface localization of Lm proteins involving diverse association systems.

AMPs are small peptides produced by living organisms [27], and constitute a major player of the innate immune response against microbial pathogens [28]. They interact with negatively charged prokaryotic surfaces, insert into the plasma membrane [27,29], and induce membrane disruption causing bacterial death [30]. Gram-positive pathogens have evolved counteracting strategies to avoid AMP-mediated killing, which include the modification of their surface charge by the D-alanylation of teichoic acids [31]. WTA glycosylations have also been shown as strategies used by Lm to resist to the action of AMPs [17,26]. Here, we show the cooperative action of several glycosylations in resistance to AMPs. While the absence of individual glycosylations (Rha and GlcNAc in Sv1/2a and Gal and Glu in Sv4b) only had a slight effect on the Lm resistance to AMPs, in both Svs, the concomitant absence of both glycosylations induced a large decrease on the Lm capacity to cope with AMPs. This could be the result of the compensatory mechanisms deployed in the absence of a single glycosylation. These results also suggest that the effect is independent from the type of glycosylation, but rather correlates with a general outcome that can be related to the decreased compactness of the cell wall and the consequent increased AMP penetration in the absence of WTA glycosylation. Indeed, WTA glycosylations appear to act mainly on the packing density and spatial constraints of the bacterial cell wall, thus modifying the kinetic of AMPs progression. This could induce some morphological alterations of the bacterial cell wall. However, our previous transmission electron microscopy analysis did not reveal any differences between the WT strain and a WTA-rhamnosylation deficient mutant [17].

We previously demonstrated that, because of their important role in the surface association of virulence factors and in resistance to AMPs, the absence of some WTA glycosylations have a strong impact on the Lm infectious capacity [17,23]. We show here that other WTA glycosylations share the same properties, however their role in virulence in vivo needs to be demonstrated.

In Bacillus subtilis and S. aureus, the loss of WTAs [32] or WTA β-GlcNAc modifications [24] renders bacteria sensitive to β-lactam antibiotics. Similarly, we found that the absence of WTA glycosylation induces an increased susceptibility of Lm to antibiotics, including ampicillin, penicillin, and gentamicin. Interestingly, as observed for AMPs, the simultaneous absence of several glycosylations induced an additional decrease in the capacity of Lm to growth in the presence of antibiotics. We can speculate that, as suggested for AMPs, this increased susceptibility to antibiotics could be due to an increased permeability of the PGN. In S. aureus, WTA-β-GlcNAc was proposed to sensitize bacteria to β-lactam antibiotics by scaffolding the proteins associated to the PGN [24], and S. aureus WTAs were shown to specifically interact with a penicillin-binding protein involved in the resistance to β-lactams [33]. In addition, WTA glycosyl substituents are also receptors for Lm phage proteins [34,35]. We thus propose that, as observed for virulence factors (Ami and InlB), WTA glycosylations could also be involved in the correct positioning of proteins involved in the decreased susceptibility to antibiotics. Most of the Lm strains are sensitive to antibiotics currently used in the treatment of human listeriosis, such as penicillin, ampicillin, and gentamicin. However, Lm strains isolated from food products appear to be resistant to some of these antibiotics [36]. Thus, it is important to analyze the role of WTA glycosylation in such resistant Lm strains.

We are currently in a race to develop new antimicrobials. While traditional antibiotics kill/inhibit the growth of bacteria, creating strong selection for resistance mechanisms [37], anti-virulence drugs disarm the pathogen without impacting its viability or growth, generating weaker resistance selection [38]. Given that the loss of most of the WTA glycosylations does not impact bacterial growth, WTA substituents hold promise for antimicrobial drug targeting. In view of their importance for pathogenesis, resistance to AMPs, and decreased susceptibility to antibiotics, this is particularly the case for Lm WTA glycosylations.

4. Materials and Methods

4.1. Bacterial Strains and Growth Conditions

The bacterial strains used in this study are described in Table 1. Listeria monocytogenes (Lm) strains were cultured in a brain heart infusion (BHI) medium (Difco), and Escherichia coli were grown in lysogeny broth (LB) media, both at 37 °C, with agitation. When necessary, the antibiotics ampicillin (amp) 100 μg/mL and erythromycin (ery) 5 μg/mL were added to select E. coli or Lm, respectively.

4.2. Construction of Deletion Mutant Strains

For this study, Lm mutant strains were constructed in a Lm Sv1/2a EGDe background through a double homologous recombination process mediated by the plasmid pMAD [39], as described in the literature [40]. DNA fragments corresponding to the upstream (UP) and downstream (DW) flanking regions of the target genes were amplified by a PCR from Lm EGDe chromosomal DNA, using specific primers 1–2 and 3–4 or 5–6, listed in Table 2.

Table 1. Bacterial strains and plasmids used in this study.

Bacterial Strains and Plasmid	Lab Code	Relevant Characteristics	Source
L. monocytogenes
EGD-e	DC 4	Wild-type; Sv 1/2a	[41]
EGD-e ∆rmlT	DC492	EGD-e rmlT (lmo1080) deletion mutant	[17]
EGD-e ∆lmo1079	DC 858	EGD-e lmo1079 deletion mutant	This study
EGD-e ∆lmo1079∆rmlT	DC 899	EGD-e lmo1079-lmo1080 deletion mutant	This study
WSLC 1042 WT	DC 825	Wild-type; Sv 4b	ATCC®23074
WSLC 1042 ∆gttA	DC 826	WSLC 1042 gttA deletion mutant	[23]
WSLC 1042 ∆gltB	DC 827	WSLC 1042 gltB deletion mutant	[23]
WSLC 1042 ∆gttA∆gltB	DC 828	WSLC 1042 gttAgltB deletion mutant	[23]
E. coli
DH5α		Competent cells	Life Technologies
Plasmid
pMAD	DC 48	Ampr and Eryr	[39]

Table 1. Bacterial strains and plasmids used in this study.

Bacterial Strains and Plasmid	Lab Code	Relevant Characteristics	Source
L. monocytogenes
EGD-e	DC 4	Wild-type; Sv 1/2a	[41]
EGD-e ∆rmlT	DC492	EGD-e rmlT (lmo1080) deletion mutant	[17]
EGD-e ∆lmo1079	DC 858	EGD-e lmo1079 deletion mutant	This study
EGD-e ∆lmo1079∆rmlT	DC 899	EGD-e lmo1079-lmo1080 deletion mutant	This study
WSLC 1042 WT	DC 825	Wild-type; Sv 4b	ATCC®23074
WSLC 1042 ∆gttA	DC 826	WSLC 1042 gttA deletion mutant	[23]
WSLC 1042 ∆gltB	DC 827	WSLC 1042 gltB deletion mutant	[23]
WSLC 1042 ∆gttA∆gltB	DC 828	WSLC 1042 gttAgltB deletion mutant	[23]
E. coli
DH5α		Competent cells	Life Technologies
Plasmid
pMAD	DC 48	Ampr and Eryr	[39]

Table 2. Primers used to amplify the flanking regions.

	Primers	Sequence (5’ → 3’) *	Restriction Enzymes
1	lmo1079 UP Fw	AGTCGGATCCGGAGCATCTTCTACATTAGGC	BamHI
2	lmo1079 UP Rv	AGTCGTCGACCCATTAACTTTCTCCCTCC	SalI
3	lmo1079 DW Fw	AGTCGTCGACTAAATGAGGGAAAACGTTAGG	SalI
4	lmo1079 DW Rv	AGTCCCATGGCACCGTGAATGAACGCC	NcoI
5	lmo1080 DW Fw	CGGGTCGACTAAGAATGGAGAGAAAAGAATGAAAGG	SalI
6	lmo1080 DW Rv	CGGCCATGGGGAATGCTTTTTCATTATAGC	NcoI
Internal Primers
7	lmo1079 Fw	GCAAATTGGAATGGGAGGCG
8	lmo1079 Rv	GGATGCCTTGTTGCCGAAAC
9	lmo1080 Fw	TATTGCCACACGCTTTACCG
10	lmo1080 Rv	CTTCCACGATTGAACGAACG
11	lmo1492 Fw	GACGGATCCCGCAACTTCGCAAAATGGG
12	lmo1492 Rv	AGCGTCGACGTCGCCATACCATCTGTTTG
pMAD Primers
13	pMAD Fw	TGATGGTCGTCATCTACCTGCC
14	pMAD Rv	CCTACGTAGGATCGATCCGACC

* Restriction sites added to the 5’ end of the primer sequence are underlined.

Table 2. Primers used to amplify the flanking regions.

	Primers	Sequence (5’ → 3’) *	Restriction Enzymes
1	lmo1079 UP Fw	AGTCGGATCCGGAGCATCTTCTACATTAGGC	BamHI
2	lmo1079 UP Rv	AGTCGTCGACCCATTAACTTTCTCCCTCC	SalI
3	lmo1079 DW Fw	AGTCGTCGACTAAATGAGGGAAAACGTTAGG	SalI
4	lmo1079 DW Rv	AGTCCCATGGCACCGTGAATGAACGCC	NcoI
5	lmo1080 DW Fw	CGGGTCGACTAAGAATGGAGAGAAAAGAATGAAAGG	SalI
6	lmo1080 DW Rv	CGGCCATGGGGAATGCTTTTTCATTATAGC	NcoI
Internal Primers
7	lmo1079 Fw	GCAAATTGGAATGGGAGGCG
8	lmo1079 Rv	GGATGCCTTGTTGCCGAAAC
9	lmo1080 Fw	TATTGCCACACGCTTTACCG
10	lmo1080 Rv	CTTCCACGATTGAACGAACG
11	lmo1492 Fw	GACGGATCCCGCAACTTCGCAAAATGGG
12	lmo1492 Rv	AGCGTCGACGTCGCCATACCATCTGTTTG
pMAD Primers
13	pMAD Fw	TGATGGTCGTCATCTACCTGCC
14	pMAD Rv	CCTACGTAGGATCGATCCGACC

* Restriction sites added to the 5’ end of the primer sequence are underlined.

The purified fragments were digested with the corresponding restriction enzymes (BamHI-SalI and SalI-NcoI) and were colligated in the multiple cloning site of the digested plasmid pMAD. The plasmid constructs were electroporated into electrocompetent Lm EGD-e cells and the transformed bacteria were selected at 30 °C in the presence of ery 5 μg/mL. Positive clones were re-isolated on a BHI-ery 5 μg/mL and incubated at 43 °C. Ery-resistant colonies were inoculated in the BHI broth at 30 °C, diluted several times, plated in BHI, and incubated overnight at 37 °C. Individual colonies were grown on BHI and BHI ery agar plates, and erythromycin-sensitive colonies were screened for the absence of the target genes using PCR with internal primers (Table 2). Both plasmid constructs and Lm gene deletions were confirmed by DNA sequencing.

4.3. Growth Analysis in Vitro

Overnight cultures of the different strains were diluted to 1:100 in fresh BHI broth, and were cultured at 37 °C with shaking. Bacterial growth was followed by measuring the optical density at 600 nm of the bacterial cultures, every 45 minutes.

4.4. Extracts of Lm Proteins

The extraction of non-covalently surface-associated and secreted Lm proteins was performed as describe before [22]. Exponential phase bacteria (20 mL, OD600 ≈ 0.8) were pelleted by centrifugation (3800 g, 15 min, 4 °C), and both the pellet and the supernatant fractions were collected. Pellets were washed with ice-cold PBS (3800 g, 10 min, 4 °C), resuspended in 200 μL of PBS + 2% sodium dodecyl sulphate (SDS), incubated (30 min at 37 °C), and centrifuged (21,000 g, 1 min). Supernatants containing the solubilized non-covalently cell surface-bound proteins were analyzed by Western blot. The culture supernatant fractions were filtered (0.22 μm) and the secreted proteins were precipitated with 0.2 mg/mL of sodium deoxycholate (DOC; 30 min, 4 °C), followed by 6% trichloroacetic acid (TCA; 2 h, 4 °C). The precipitated proteins were recovered by centrifugation (13,400 g, 15 min, 4 °C) and were washed twice with cold acetone (100%). The pellet was air-dried and resuspended in 200 μL of 20 mM Tris-HCl, pH 7.4, for the Western blot analysis.

4.5. SDS-PAGE and Western Blot Analysis of Protein Extracts

Lm protein extracts were resolved by SDS-PAGE in an 8% polyacrylamide gel. The proteins were transferred (Trans-Blot Turbo Transfer System; Bio-Rad Laboratories) onto a nitrocellulose membrane, according the manufacturer’s guidelines. Nitrocellulose membranes were stained with Ponceau S for loading control and were blocked in Buffer A (20 mM Tris-HCl, 0.9% NaCl, pH = 7.4) with 0.1% tween and 5% skimmed milk. The membranes were incubated overnight at 4 °C with a primary antibody diluted in Buffer A with 0.1% tween and 2.5% skimmed milk—mouse monoclonal anti-InlB (A13.1 [42]; (1:2000)), rabbit polyclonal anti-Ami antiserum (R5, from Pascale Cossart, Institut Pasteur; 1:5000), and rabbit polyclonal anti-Lm Glyceraldehyde-3-phosphate dehydrogenase (GAPDH) (Abgent; 1:100). The membranes were probed with anti-mouse or anti-rabbit horseradish peroxidase (HRP)-conjugated secondary antibodies (1:2000; P.A.R.I.S Biotech) in Buffer A with 0.1% tween and 2.5% skimmed milk. The signals were detected by chemiluminescence using a PierceTM Western Blotting Substract kit (Thermo Fisher Scientific) under ChemiDoc XRS + equipment (Bio-Rad Laboratories).

4.6. Antimicrobial Peptides Susceptibility

WTA glycosylation deficient strains and isogenic wild type strains were tested for their susceptibility to LL-37 or CRAMP (AnaSpec), as described in the literature [17]. Briefly, bacteria in the exponential phase of growth (OD600 ≈ 0.8) were diluted to 10⁴ CFU/mL in a sterile phosphate buffer (PB) medium (10 mM phosphate buffer, pH 7.4; 1% BHI). Bacterial suspensions were incubated with CRAMP or LL-37 in a 96-well microplate (2 h at 37 °C), without shaking, serially diluted in sterile phosphate buffer solution (PBS), and plated in BHI agar for the quantification of viable bacteria. As the control, bacterial suspensions without AMPs were used. For growth analysis in the presence or absence of AMPs, Lm strains in the exponential phase of growth (OD600 ≈ 0.8) were diluted (10⁷ CFU/mL) in a sterile PB medium in a 96-well microplate, and incubated with or without CRAMP or LL-37 for 4 h at 37 °C with shaking. The optical densities at 600 nm were measured every 15 minutes using the Synergy2 equipment (BioTek). Solutions containing only AMPs were used for background subtraction.

4.7. Antibiotic Susceptibility

The susceptibility to antibiotics of Lm strains was assessed by measuring the MICs through the E-test method (

Table 3. Range of antibiotic concentrations tested against Lm.

Antibiotic	Strip Concentration (μg/mL)
Gentamicin Ampicillin Benzylpenicillin	0.016-256 0.016-256 0.002-32

). Bacteria in the stationary phase were inoculated at a high density on Mueller Hinton (MH) agar (Sigma-Aldrich) plates with a sterile cotton swab. ETEST® strips (BioMérieux) of each antibiotic (Table 3) were applied on the inoculated plates before overnight incubation at 37 °C. The day after, the susceptibility halos were analyzed as recommended.

4.8. Statistical Analysis

Statistical analyses were carried out with Prism software (GraphPad) using one-way ANOVA with Dunnett’s post hoc analyses to compare different means in relation to a control sample, and Tukey’s post hoc analyses for pairwise comparisons of more than two different means. A two-tailed unpaired Student’s t-test was used for a comparison of the means between two samples. For statistically significant differences: * p ≤ 0.05; ** p ≤ 0.01; *** p ≤ 0.001; **** p ≤ 0.0001.