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Article

Selection of Lactiplantibacillus Strains for the Production of Fermented Table Olives

by
Teresa Zotta
1,
Marilisa Giavalisco
1,
Eugenio Parente
1,*,
Gianluca Picariello
2,
Francesco Siano
2 and
Annamaria Ricciardi
1
1
Scuola di Scienze Agrarie, Alimentari, Forestali ed Ambientali (SAFE), Università degli Studi della Basilicata, 85100 Potenza, Italy
2
Istituto di Scienze dell’Alimentazione-CNR, 83100 Avellino, Italy
*
Author to whom correspondence should be addressed.
Microorganisms 2022, 10(3), 625; https://doi.org/10.3390/microorganisms10030625
Submission received: 24 February 2022 / Revised: 10 March 2022 / Accepted: 11 March 2022 / Published: 15 March 2022
(This article belongs to the Special Issue Microorganisms and Fermented Foods)
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Abstract

:
Lactiplantibacillus strains (n. 77) were screened for technological properties (e.g., xylose fermentation, EPS production, antimicrobial activity, tolerance to NaCl and phenolic compounds, oleuropein degradation and hydroxytyrosol formation) relevant for the production of fermented table olives. Survival to olive mill wastewater (OMW) and to simulated gastro-intestinal tract (GIT), the capability to grow at different combinations of NaCl and pH values, radical scavenging activities and biofilm formation were further investigated in 15 selected strains. The screening step revealed high diversity among Lactiplantibacillus strains. Most of the strains were able to ferment xylose, while only a few strains produced EPS and had inhibitory activity against Y. lipolytica. Resistance to phenolic compounds (gallic, protocatechuic, hydroxybenzoic and syringic acids), as well as the ability to release hydroxytyrosol from oleuropein, was strain-specific. OMWs impaired the survival of selected strains, while combinations of NaCl ≤ 6% and pH ≥ 4.0 were well tolerated. DPPH and hydroxyl radical degradation were strain-dependent, while the capability to form biofilm was affected by incubation time. Strains were very tolerant to the GIT. The genome of Lpb. pentosus O17 was sequenced and analysed to verify the presence of genes involved in the degradation and metabolism of phenolic compounds. O17 lacks carboxylesterase and gallate decarboxylase (subunits B and D) sequences, and its gene profile differs from that of other publicly available Lpb. pentosus genomes.

1. Introduction

Lactiplantibacillus paraplantarum, Lpb. plantarum and Lpb. pentosus (formerly Lactobacillus paraplantarum, Lb. plantarum and Lb. pentosus [1]) are three phylogenetically close species [1] involved in several food, biotechnological and health-related applications. Strains belonging to the Lactiplantibacillus group have a wide ecological distribution (e.g., presence in vegetable, cereal, meat and dairy products, as well as human hosts) and are characterized by high phenotypic and genomic diversity. Lactiplantibacillus genomes, in fact, are large (from 2.9 to 5.3 Mbp; NCBI database), and comparative genome and pangenome analyses revealed the presence of accessory and unique (strain-specific) genes consistent with the evolution and adaptation to different ecological niches, confirming the versatility of this group [2,3,4].
Strains of the Lactiplantibacillus group are important members of olive surface microbiota [5,6] and, thus, they can play a crucial role in the production of olive-derived products. Fermented table olives can be processed with different methods: drupes can be debittered through an alkaline treatment (NaOH 2.5–3% w/v) and then fermented in brine (NaCl 10–11% w/v) for 3–7 months (treated table olives, Spanish style); alternatively, olives can be fermented directly in brine (NaCl 6–10% w/v) for 8–12 months, with a debittering process driven by the enzymatic activities of indigenous microorganisms (natural table olives, Greek style; see Perpetuini et al. [5] for more details).
Lactiplantibacillus strains may dominate the spontaneous fermentation [7,8,9] of several types of table olives, or they may be deliberately added as starter and adjuncts, alone or in combination with yeasts, to control and standardize the fermentative process [5,10,11]. Lactiplantibacillus starters may reduce the fermentation time, and may improve the organoleptic (e.g., debittering, aroma profile, pulp and colour stability), nutritional (e.g., antioxidant compounds) and microbiological quality (e.g., the acidification of brine and antimicrobial compounds may prevent spoilage and pathogens) of table olives [5].
The survival of strains (naturally present or deliberately added) during the fermentative process (both in Spanish- and Greek-style olives) depends on several factors (e.g., low pH, high concentrations of salt and phenolic compounds and competition with other species) and, therefore, the capability to cope with multiple stresses is essential for their fitness during fermentation and for obtaining stable and high-quality products.
The presence of high phenolic compound levels is certainly one of the main constraints in olive fermentation. Members of the Lactiplantibacillus group are able to degrade and use several phenolic compounds (e.g., gallic, p-coumaric, ferulic, protocatechuic acids and oleuropein), although this feature is strain-dependent and has been often investigated in in vitro studies (i.e., in synthetic media containing phenolic compounds) [12]. Moreover, many studies have addressed the response to single phenolic compounds, but it is known that olives are a complex phenol-rich matrix in which the synergic effect of different phenolic fractions may exacerbate their antimicrobial activity. In brines, additionally, the resistance to phenolic compounds (released in aqueous phase) is also affected by the presence of high salt concentrations and low pH values [13]. The metabolism of phenolic compounds in the Lactiplantibacillus group is related to the activity of several degrading enzymes (e.g., β-glucosidase, esterase, tannase, decarboxylases), and the occurrence of genes coding for these enzymes may be a criterion for the selection of strains. To date, the occurrence of genes has been mainly evaluated in Lpb. plantarum strains and, to a lesser extent, in Lpb. pentosus [14,15,16,17,18], although this species is frequently isolated and associated with olives and their derived products [5,13].
In this study, we tested a collection of Lactiplantibacillus strains (n. 77, isolated from different sources) for technological properties (i.e., xylose fermentation, EPS, GABA and catalase production, antimicrobial activity, tolerance to NaCl and phenolic compounds, oleuropein degradation and hydroxytyrosol formation) useful for the production of fermented olives. Particular efforts focused on the tolerance against phenolic compounds, including the survival in olive mill wastewater (selected as a model of a phenol-rich matrix). The genome of Lpb. pentosus O17 (the most tolerant and promising strain) was sequenced and analysed to verify the occurrence of genes involved in the degradation and metabolism of phenolic compounds, and the gene profile was compared with that of other publicly available Lpb. pentosus genomes.

2. Materials and Methods

2.1. Strains and Culture Conditions

Seventy-seven strains of Lactiplantibacillus paraplantarum (n. 4), Lpb. plantarum (n. 50) and Lpb. pentosus (n. 23) were used in this study (Table 1). The strains were isolated from different sources and maintained as freeze-dried stocks (11% w/v skim milk with 0.1% w/v ascorbic acid) in the Culture Collection of Industrial Microbiology Laboratory, Università degli Studi della Basilicata. Lactobacilli were propagated (16 h, 30 °C) in Weissella Medium Broth pH 6.8 (WMB [19]) before each assay.
The strains Debaryomyces hansenii DH-02, Yarrowia lipolytica YL-12, Listeria innocua BL86/26 and Lpb. plantarum C17 were used as indicators for the deferred antagonism assay (Section 2.3). D. hansenii and Y. lipolytica were routinely cultivated (24 h, 25 °C) in yeast extract–Peptone–dextrose broth (YPD broth), L. innocua in tryptone soya broth supplemented with 6 g/L yeast extract (TSBYE; 24 h, 30 °C) and Lpb. plantarum C17 in WMB (16 h, 30 °C).

2.2. Identification of Lactiplantibacillus Strains Isolated from Olives and Brines

Sixty-five strains were already present in the Culture Collection of Industrial Microbiology, while twelve Lactiplantibacillus (* in Table 1) were isolated, in this study, from natural and cured (NaOH treatment) table olives and the brines of Bella di Cerignola and Cellina di Nardò (Puglia, Italy) cultivars. Specifically, 24 isolates were recovered (30 °C, 24 h, anaerobiosis) on modified MRS agar (mMRS) supplemented with 0.02 g/L bromophenol blue and 0.5 g/L cysteine (for colony morphology [20]) and with 100 mg/L cycloheximide (to inhibit growth of yeasts and moulds). Specifically, light-blue colonies with dark-blue centres (morphology of Lactiplantibacillus strains on mMRS [20]) were collected and purified before taxonomic identification.
Genomic DNA was extracted from each isolate by using the GeneElute Bacterial Genomic DNA Kit (Sigma-Aldrich, St. Louis, MO, USA) and quantified with a NanoDrop 1000c spectrophotometer (Thermo Scientific, Wilmington, DE). Isolates were de-duplicated using RAPD-PCR (primer M13 [21]) and identified at species levels through amplification (Table S1) and sequencing (external service, Genechron Srl, Roma, Italy) of the 16S rRNA gene and with a multiplex PCR assay (amplification of recA gene [22]).

2.3. Technological Characterization of Lactiplantibacillus Strains: A Screening Step

All strains were tested for technological features that could be useful for the production of fermented table olives and for other applications related to olive-derived products.
Xylose fermentation: WMB cultures were plated on MRS agar containing 10 g/L D-xylose and 0.16 g/L bromocresol purple (BCP) as the pH indicator, and incubated at 30 °C for 48 h under anaerobic conditions. The change of substrate colour from purple to yellow and the presence of yellow colonies indicated the ability to use xylose.
Tolerance of high NaCl concentrations: WMB cultures were standardized to a final absorbance at 650 nm (A650) of 1.0 (Bio-Rad Smart Spec™ Plus, Bio-Rad Laboratories Inc.) and used to inoculate (10% v/v) WMB supplemented with 7.5% w/v or 10% w/v NaCl and 0.16 g/L BCP. After incubation (30 °C, 48 h, anaerobiosis) the change of colour from purple to yellow indicated the presence of survivors.
Production of exopolysaccharides (EPS): the strains were screened for EPS production by using a pick test on MRS agar plates containing 20 g/L maltose (M-MRS) or 20 g/L glucose (G-MRS) or 50 g/L sucrose (S-MRS) as carbon sources. At the end of incubation (30 °C, 24 h, anaerobiosis), the strains which produced translucent slimy or ropy colonies were recorded as EPS producers.
Production of γ-amino butyric acid (GABA): WMB cultures were standardized (absorbance at 650 nm, A650 of 3.0) and used to inoculate (1% v/v) WMB with or without 1% (w/v) monosodium glutamate (MSG). At the end of incubation (30 °C, 24 h, anaerobiosis), pH values (CyberScan pH11/110, Oakton Instruments, Vernon Hills, USA; Double Pore Slim electrode, Hamilton Company, Reno, NV, USA) and A650 were measured, and the supernatants were collected (12,000× g, 5 min, 4 °C). The accumulation of GABA in unsupplemented WMB and WMB-MSG was qualitatively evaluated by thin layer chromatography (TLC; silica gel plates, cod. Z292974-1PAK, Sigma-Aldrich, St. Louis, MO, USA). The mobile phase was a mixture of n-butanol, acetic acid and deionized water (4:1:1 ratio), supplemented with 0.2% (w/v) ninhydrin for spot detection (red-purple colour). Samples were loaded (1.5 µL/spot) on TLC plates and separated in a TLC chamber at room T°C; after the run, the TLC plates were heated at 70 °C for spot visualization. WMB supplemented with 1% (w/v) MSG or GABA were used as controls.
Antimicrobial activity: inhibitory activity was tested by using a deferred antagonism assay, as described in Parente et al. [23]. All lactobacilli were spotted (5 μL) on MRS agar plates and incubated at 30 °C for 48 h. The overlay soft-agar (0.6% w/v) media containing the indicator strains were YPD for D. hansenii DH-02 and Y. lipolytica YL-12, TSBYE for L. innocua BL86/26 and buffered MRS (0.1 mol/L MOPS) for Lpb. plantarum C17. At the end of incubation (24 h, 30 °C), the diameter of the inhibition zones around spots were measured using a calliper.
Catalase activity: the catalase activity of lactobacilli cultivated in unsupplemented and heme-supplemented WMB was qualitatively detected (bubble formation) as reported by Zotta et al. [24].
Resistance to phenolic compounds: the strains were cultivated (30 °C, 24 h) in modified WMB pH 6.5 containing 2 g/L of ribose as a carbon source (mWMB), washed twice with NaCl 0.85% (w/v), standardized to an A650 of 1.0 and used to inoculate (10% v/v; 96-well-microplate experiments) mWMB supplemented with gallic acid (two-fold dilution from 100 to 6.25 mM), protocatechuic acid (from 50 to 3.12 mM), 4-hydroxybenzoic acid (from 40 to 2.5 mM) and syringic acid (from 25 to 1.56 mM). After incubation (30 °C, 24 h), the substrate turbidity (semi-quantitative assay) indicated the presence of survivors at a given concentration of phenolic compound.
Hydrolysis of oleuropein and production of hydroxytyrosol: standardized mWMB cultures (as above) were used to inoculate (10% v/v) 96-well microplates containing MRS pH 7.4 (without meat extract [25]) supplemented with 1 g/L oleuropein. At the end of incubation (7 days, 30 °C, anaerobiosis), the supernatants were collected (12,000× g, 5 min, 4 °C) and the oleuropein degradation and hydroxytyrosol formation were qualitatively evaluated through a TLC assay, as described by Ciafardini et al. [25], with some modifications. Briefly, the mobile phase was a mixture of n-propanol: benzyl alcohol: 88%; formic acid: water (50:72:20:20 ratio). Samples were loaded (1.5 µL/spot) on TLC plates, and separated in a TLC chamber at room T°C. After the run, the TLC plates were dipped in Folin–Ciocâlteu 30% (v/v) and air-dried at room T°C for spot visualization (grey-brown colour). MRS pH 7.4 supplemented with oleuropein or hydroxytyrosol (0.25 g/L final concentration) were used as controls. For each assay, two biological replicates were carried out.

2.4. Characterization of Selected Lactiplantibacillus Strains

Fifteen strains (Lpb. pentosus OM13, OM14, OM24, OM50, OM53, OM52, OM62, 2TP, O17 and O18; Lpb. plantarum subsp. plantarum C17, ISLCPT57, MT2A11S and WCFS1; Lpb. plantarum subsp. argentoratensis MTC13L) were selected on the basis of previous assays, routinely cultivated in WMB (30 °C, 24 h) and used to verify for the following properties:
Radical scavenging activity: the capability to remove 1,1-diphenyl-2-picrylhydrazil (DPPH) and hydroxyl radicals was measured on standardized cells (A650 = 1.0), as described by Wang et al. [26]. For both assays, two biological replicates were carried out.
Biofilm formation: standardized cells (A650 = 1.0) were used to inoculate 96-well (flat-bottomed) polystyrene microplates, filled with WMB pH 6.8. After 24 and 48 h of incubations at 30 °C, supernatants and non-adherent cells were removed by inverting the plates, and biofilms were stained with 200 μL of crystal violet (0.1% w/v) for 30 min at 30 °C ([27], with some modifications). At the end of the incubation, the excess dye was discarded and gently washed (3 times) with phosphate buffer 20 mM pH 7.0 (PB7). Crystal violet was solubilized in 200 μL of 96% (v/v) ethanol, and absorbance at 595 nm (A595) was measured with a microplate reader (SPECTROStar Nano; BMG Labtech, Ortenberg, Germany). Three biological replicates were carried out.
Resistance to different combinations of NaCl and pH values: standardized cells (A650 = 1.0) were used to inoculate (10% v/v; 96-well microplates) WMB with different combinations of NaCl (0, 4.0, 6.0 and 8.0% w/v) and pH (6.0, 5.0, 4.0 and 3.0) values. WMB pH 6.0, without salt, was used as the control. After 24 and 48 h of incubations at 30 °C, A650 values were measured with a microplate reader. Two biological replicates were carried out.
Resistance to simulated gastro-intestinal tract: standardized cells (A650 = 1.0) were re-suspended in simulated saliva (SS; 25 mM NaCl, 7 mM KCl, 45 mM NaHCO3, 100 mg/L lysozyme pH 6.9 [28]) and incubated at 100 rpm (SW20 shaking thermostatic water bath, JULABO GmBH, Seelbach, Germany) for 5 min at 37 °C. At the end of the incubation, cells were harvested (8000× g, 10 min, 4 °C), re-suspended in simulated gastric juice (SGJ; 25 mM NaCl, 7 mM KCl, 45 mM NaHCO3, 0.3 g/100 mL pepsin, pH 3.0 [29]) and incubated at 100 rpm for 1 h at 37 °C. SGJ-treated cells were then collected, re-suspended in simulated pancreatic juice (SPJ; 0.15 g/100 mL bile salt, 0.1 g/100 mL trypsin, 0.1 g/100 mL α-chymotrypsin, pH 8.0 [29]) and incubated at 100 rpm for 1 h at 37 °C. Untreated cells, incubated in PB7, were used as controls. The numbers of survivors were enumerated in each step (SS, SGJ and SPJ) by pour plating on WMB agar (30 °C, 48 h, anaerobiosis). Two biological replicates were carried out.
Survival in olive mill wastewater: Olive mill wastewaters (OMWs) obtained from the olive oil production of Leccino, Coratina (oil mill located in Tricarico, Basilicata region, Italy) and Cima di Melfi (olive oil mill located in Grottaglie, Puglia region, Italy) cultivars were treated at 90 °C for 15 min and centrifuged (2800× g, 15 min, 20 °C) to remove solid residues. The effectiveness of heat treatment was verified via plate counting on different substrates (mMRS agar with 100 mg/L cycloheximide and 15 mg/L nalidixic acid, 48 h at 30 °C for detection of lactic acid bacteria (LAB); glucose–yeast extract–agar, GYEA, with 100 mg/L chloramphenicol, 30 °C at 48 h for yeasts and 5 days for moulds; VRBGA, 24 h at 30 °C for Enterobacteriaceae; gelatine peptone agar, 72 h at 30 °C for total aerobic count).
The strains were standardized and inoculated (final population of 107 ufc/mL) in different concentrations (two-fold dilution from 50% to 0% v/v; 96-well-microplate experiments) of OMWs for 15 min at 30 °C. At the end of the incubation, OMW-treated cells were inoculated (10% v/v) in WMB broth pH 6.8 to evaluate the presence of survivors (substrate turbidity; semi-quantitative assay) after 24 h of incubation at 30 °C.
The strains with the highest resistance (Lpb. pentosus OM24 and O17, Lpb. plantarum C17 and MT2A11S) were further investigated for their tolerance to OMW (from 50% to 0% v/v) by using longer incubation times (15, 30, 60 and 120 min, at 30 °C). Survivors were evaluated as described before. For each assay, two biological replicates were carried out.

2.5. Total Phenolic Content and Phenolic Profile of OMW

OMW supernatants (3000× g, 15 min, 4 °C) of Leccino, Coratina and Cima di Melfi cv. (Section 2.5) were filtered (Millex® filter 0.22 µm, Merck-Millipore, Billerica, MA, USA) and used for the detection of total phenolic content (TPC; Folin–Ciocâlteu assay) and the analysis of the phenolic profile (PP; HPLC-DAD).
For TPC, 50 µL of 40-fold-diluted filtered OMWs was combined with 2.3 mL deionized water and 50 µL Folin–Ciocâlteu 50% (v/v), and, after 3 min, 100 µL of saturated sodium carbonate was added. Mixtures were incubated in the dark at room T°C for 90 min. At the end of the incubation, absorbance at 765 nm (A765) was measured. A calibration curve (R2 > 0.99) with different concentration of gallic acid (from 0.05 g/kg to 0.5 g/kg) was used to quantify the TPC. The results were expressed as grams of gallic acid equivalent (GAE) per kilogram of OMW (g GAE/kg of OMW). Three technical replicates were performed for each sample.
For HPLC analysis, the filtered OMWs were 40-fold diluted with 0.1% (v/v) trifluoroacetic acid (TFA), and the phenolic compounds were separated using a modular chromatograph HP1100 (Agilent Technologies, Paolo Alto, CA, USA) equipped with a reverse phase C18 column, 250 × 2.0 mm i.d., 4 mm particle diameter (Jupiter Phenomenex, Torrance, CA, USA). The column temperature was held at 40 °C during the HPLC analysis. Analyses were performed at a constant flow rate of 0.2 mL/min, applying the following gradient of solvent B (acetonitrile/0.1% v/v TFA): isocratic elution at 5% of B for 5 min, and linear gradient 5–60% of B for 5–65 min and 60–100% of B at 65–70 min. Solvent A was 0.1% TFA in HPLC-grade water. For each run, 100 μL of diluted samples was injected. Analyses were performed in triplicate and monitored at 520, 360, 320, 254 and 280 nm, also acquiring the UV-Vis spectrum every second in the 200–600 nm range with a diode array detector (DAD). The main peaks were assigned according to the order of elution [30], matching the UV-Vis spectra with those of pure phenolics, with matches confirmed with authentic standard compounds if available. The oleuropein derivative was confirmed through the HPLC monitoring of its disappearance and the release of hydroxytyrosol upon acidic hydrolysis (3N HCl, 40 °C, 3 h). Chromatograms were analysed by using the Chem Station vers A.07.01 HPLC software (Agilent Technologies, Santa Clara, CA, USA).

2.6. Genome Sequencing of Lactiplantibacillus pentosus O17 and Occurrence Analysis of Genes Involved in Degradation and Metabolism of Phenolic Compounds

The whole genome of Lpb. pentosus O17, the strain with the best tolerance, was sequenced (WGS) by using an Illumina NovaSeq 6000 platform (IGA Technology s.r.l., Udine, Italy). The reads were de novo assembled using SPAdes v.3.14, while the functional annotation was performed using the NCBI Prokaryotic Genome Automatic Annotation Pipeline (PGAP). The WGS project was deposited at GenBank under the accession number JAHLCJ000000000.1 (https://www.ncbi.nlm.nih.gov/nuccore/JAHLCJ000000000.1 accessed on 15 January 2022).
The WGS of Lpb. pentosus O17 was analysed to verify the occurrence (presence, absence) of genes involved in the degradation and metabolism of phenolic compounds: β-glucosidase (also annotated as 6-phospho-β-glucosidase), gallate decarboxylase (subunits B, C, D), p-coumaric acid decarboxylase (also annotated as phenolic acid decarboxylase), esterase (also annotated as acetyl esterase/lipase or alpha/beta hydrolase), carboxylesterase, tannase (subunits A and B) and the transcriptional regulator PadR. The genes of interest were identified on the basis of data available in literature (see Table S2).
Gene profile of Lpb. pentosus O17 was compared with that of 28 Lpb. pentosus genomes retrieved from Integrated Microbial Genome database (IMG; https://img.jgi.doe.gov/cgi-bin/mer/main.cgi; accessed on 15 January 2022).

2.7. Statistical Analysis

Statistical analyses and graphs were obtained using Systat 13.0 for Windows (Systat Software Inc., San Jose, CA, USA) and R 4.1.2 [31].

3. Results and Discussion

3.1. Identification and Technological Characterization of Lactiplantibacillus Strains

In this study, a collection of Lactiplantibacillus strains were tested for some technological properties useful for the production of fermented table olives. The strains came from different isolation sources (Table 1) in order to verify possible correlations between functionality and ecological niches of isolation. In this study, 24 isolates were recovered from olives and brines, and multiplex PCR and partial 16S rRNA gene sequencing confirmed their membership to Lpb. plantarum (n. 3) and Lpb. pentosus (n. 9) species.
All strains (with the exception of Lpb. plantarum O4) were able to grow in the presence of xylose (Figure 1), but only 27 were able to produce acid. This feature was widespread among isolates from olives (85%), although some strains from sourdoughs (i.e., MTNTA3S and MT2A11S) and wine (i.e., UBS3) also fermented xylose. This pentose is a hemicellulose-derived sugar present in several plant materials, including olive pulp, stones and pomace [32]. Therefore, the capability to use it may be of practical relevance in the production of olive-derived products. Additionally, D-xylose may be used to discriminate Lactiplantibacillus species, as the strains of Lpb. paraplantarum are unable to ferment it [33].
The ability to tolerate high salt concentrations is another relevant feature for the production of fermented olives. Several table olives (e.g., green Spanish style, black Greek style), in fact, are produced with brines containing from 4 to 12% of NaCl, which is useful to prevent spoilage and modify the organoleptic properties of drupes [5,11]. On the other hand, the salt concentration in brines significantly affects olive microbiota, increasing the relative abundance of yeasts compared to LAB at NaCl levels above 8% [6].
In this study, no strains were able to grow in the presence of 10% NaCl, while most of them (n. 58, mostly from olives and brines; Figure 1) grew with 7.5% NaCl. Lpb. paraplantarum strains, however, were very sensitive to salt, and were unable to grow at 7.5% NaCl. Several authors [25,34,35,36,37,38] have demonstrated that salt concentrations higher than 10% NaCl were detrimental for many Lactiplantibacillus strains, while lower levels (synthetic media supplemented with ≤ 7–8% NaCl) were well tolerated.
Sixteen strains (69% were from sourdoughs) produced EPS from both glucose, maltose and sucrose; Lpb. pentosus O18 formed EPS only from maltose, while Lpb. pentosus O19, OM50 and OM53 formed EPS only from sucrose (Figure 1; Table S3). No strain was able to produce dextran. The EPS from LAB may be used in the food industry as stabilizers, emulsifiers or gelling agents as they affect the rheological properties and texture of foods [39]. EPS, moreover, can be involved in adhesion and biofilm formation, improving the colonization ability of strains. EPS production in Lactiplantibacillus strains, then, may be beneficial to guarantee their permanence on olive fruits during fermentation.
The Lactiplantibacillus strains screened in this study did not show antagonistic activity against Lpb. plantarum, D. hansenii (members of olive microbiota [40]) and L. innocua (used as a proxy for L. monocytogenes, a pathogen possibly presents in table olives, especially under reduced salt fermentation [41,42]). Only 15 strains had inhibitory activity against Y. lipolytica (associated with olive microbiota; see Figure 1 and Table S3). The antimicrobial activity of Lactiplantibacillus isolated from olives (like other LAB) is related to the production of bacteriocins and organic acids [11,43,44], but these features are strongly affected by fermentation conditions (e.g., T°C, pH, salt concentrations [11]).
In this study, none of the strains were able to produce GABA when cultivated in the presence of sodium glutamate, while most of them (71, 92.2%) were able to synthesize heme catalase, the main H2O2-degrading enzyme in LAB.

3.2. Tolerance and Degradation of Phenolic Compounds

Olives and their derived products are phenolic-rich matrices, and the assessment of strain survival is crucial for the development of competitive cultures. Phenolic compounds detected in olives mainly include hydroxycinnamic (caffeic, p-coumaric, o-coumaric, ferulic and sinapic) and hydroxybenzoic (gallic, 4-hydroxybenzoic, protocatechuic, syringic and vanillic) acids, as well as phenolic alcohols, such as tyrosol and hydroxytyrosol [12,45].
In this study, only 19 strains (mostly Lpb. pentosus from olives) were able to grow in the presence of 100 mM gallic acid, while most strains (n. 73) grew in media supplemented with 50 mM protocatechuic acid and (n. 66) 25 mM syringic acid (Figure 1). Hydroxybenzoic acid had the highest toxicity, and none of the strains were able to grow at the highest concentration (40 mM). On the contrary, lower levels of phenolic acids (gallic ≤50 mM, protocatechuic ≤25 mM, hydroxybenzoic ≤20 mM and syringic ≤12.5 mM) did not inhibit the growth of strains. The analysis of the minimum inhibitory concentration (MIC) grouped the strains into three different clusters (Figure 2): the first one (C1) included strains with the lowest tolerance to phenolic compounds; the second large group (C2) included strains able to cope with the highest levels of protocatechuic (50 mM) and syringic (25 mM) acids, but unable to tolerate high concentrations of gallic (100 mM) and 4-hydroxybenzoic (40 mM) acids; the third cluster (C3) grouped the most tolerant lactobacilli (isolated from olives and sourdoughs), characterized by their greater resistance to gallic acid (100 mM).
As already demonstrated [12], we confirmed that the capability of the Lactiplantibacillus group to survive to olive-associated phenols is strain-specific; however, compared to other studies in which a limited number of strains has been tested, in this work, a relatively large collection of strains was considered, improving the information on the functional diversity of the Lactiplantibacillus group.
Oleuropein, the secoiridoid glycoside that causes the bitter taste of olives, is another important phenolic compound, and its degradation is essential to make olives and their derived products edible for humans. Oleuropein is hydrolysed into glucose and aglycone by β-glucosidases of both endogenous (olive fruit) or exogenous (microbial) origin. In turn, oleuropein aglycone is converted into elenolic acid and hydroxytyrosol (non-bitter compounds) through the activity of an esterase enzyme or, in part, through acidic hydrolysis. Ligstroside, which differs from oleuropein only because the tyrosol replaces the hydroxytyrosol moiety, undergoes a similar fate to oleuropein.
In this study, the capability to degrade oleuropein (TLC assay; Figure S1) was widespread among the strains (n. 71; β-glucosidase activity), while the capability to release hydroxytyrosol (esterase activity) was found only in 50 lactobacilli (Figure 1; Table S4). The source of isolation, however, did not affect oleuropein degradation and hydroxytyrosol formation, as these features were also found in strains isolated from matrices other than olives and brines (Figure 1). Similar to our results, Zago et al. [36] found that some Lpb. plantarum strains isolated from several cheeses were able to hydrolyse oleuropein. The hydrolysis of oleuropein has been studied for a long time in the Lactiplantibacillus group [6,7,12,25,46], and it is well known that this feature is strain-dependent.
During olive fermentation (especially for non-alkali treated fruits), Lactiplantibacillus starters may reduce the oleuropein content [47], debittering the final product and increasing the hydroxytyrosol level. Ramírez et al. [48] demonstrated that the degrading ability of Lpb. plantarum and Lpb. pentosus strains was significantly different, and only a few strains were able to hydrolyse most of the oleuropein (up to 90% of initial concentration) added to the reaction medium. This underlines that the debittering capability of Lactiplantibacillus strains (besides the presence of β-glucosidase and esterase activities) may also be affected by oleuropein content, which in turn is related to the olive cultivars [49]. More recently, Vaccalluzzo et al. [6] found that the oleuropeinolytic activity of Lpb. plantarum strains was affected by a low temperature, rather than high salt concentrations and low pH values.
Oleuropein, moreover, may affect the functionality of the starter cultures regulating the transcriptional levels of genes involved in the growth, transport, carbohydrate metabolism, bacteriocin production and quorum sensing of Lpb. plantarum [50]; therefore, the capability to degrade and use it is crucial for the selection of functional and competitive cultures.
The ability to form hydroxytyrosol is a desired feature among Lactiplantibacillus strains, as it may improve the antioxidant properties of olive-derived products, providing benefits for human health; free hydroxytyrosol, in fact, is one of the most powerful free radical scavengers, and it is also a metal chelator, exerting potential cardioprotective, anticancer, endocrine regulator and antimicrobial effects (in vitro and in vivo trials, however, demonstrated that the potential benefits are related to both dose and timing of intake [51,52]). To this purpose, EFSA indicated that the consumption of olive oil containing hydroxytyrosol or tyrosol as well as their derivatives (daily intake of 5 mg Hyt/20 g olive oil) helps to protect blood lipids from oxidative stress (Commission Regulation EU n.432/2012).

3.3. Characterization of 15 Selected Lactiplantibacillus Strains

The capability to scavenge radicals, to form biofilm, to grow in the presence of different NaCl concentrations and pH values, to survive in phenolic-rich matrices and to simulate the gastro-intestinal tract (GIT) was investigated in 15 selected strains (* in Figure 1 and Figure 2). The strains were chosen mainly on the basis of phenolic compound tolerance, but other features (e.g., salt tolerance, oleuropein degradation and hydroxytyrosol formation, as well as EPS production) were also considered. Lpb. plantarum subsp. plantarum ISLCPT57, which lacked most of these important properties, was included for comparison.
A wide variability among Lactiplantibacillus strains was observed in hydroxyl radical scavenging activity (ranging from 60% for Lpb. pentosus O17 to 8% for Lpb. plantarum subsp. plantarum ISLCPT57; Figure 3). On the contrary, although the capability to remove DPPH radicals ranged from 40% (Lpb. pentosus O17) to 10% (Lpb. plantarum subsp. plantarum ISLCPT57), most of the strains exhibited comparable detoxification activity. In both cases, Lpb. pentosus O17 exhibited the highest scavenging ability.
LAB are able to scavenge toxic radicals by producing different antioxidant enzymes (i.e., superoxide dismutase, catalase, flavin-dependent oxidases/peroxidases, thioredoxin and glutathione reductases). Radical scavenging activity may prevent oxidative processes in foods, ensuring the stability of proteins, lipids and phenolic compounds.
Kachouri et al. [53] demonstrated that a Lpb. plantarum strain with radical scavenging properties increased the phenolic content and total antioxidant activity of Chetoui olives during the storage period. The beneficial effect of antioxidant strains was evaluated also in other olive-derived products; some authors [54,55], for example, demonstrated that virgin olive oil produced with fruits inoculated with Lpb. plantarum had higher total phenolic content and greater stability to oxidative processes than that obtained from uninoculated drupes. The use of Lpb. plantarum, moreover, increased the antioxidant activity of OMW [56], reducing the auto-oxidation of phenolic compounds.
In this study, the potential capability to form stable biofilms (CV assay) was also evaluated. The A595 values (Figure 4) differed among the strains and, for most of them, were dependent on incubation time; prolonged cultivation (48 h), in fact, increased (by 1.6 and 7.1 times, respectively, for Lpb. pentosus OM52 and OM53) the fraction of adherent cells compared to 24 h of incubation. Lpb. pentosus O17 and Lpb. plantarum MT2A11S exhibited the highest ability in biofilm formation after both 24 and 48 h of growth, while Lpb. plantarum subsp. plantarum ISLCPT57 had the lowest fraction of adherent cells. In this study, the capability to form biofilm was not correlated to EPS production ability, since some of the best biofilm producers (e.g., Lpb. pentosus O17, Lpb. plantarum MT2A1 and WCFS1) were unable to synthetize EPS from the sugars used in the screening step (see Table S3).
During the olive fermentation process, Lactiplantibacillus strains were able to shape a compact biofilm on both biotic (olives skin) and abiotic (glass slides) surfaces to ensure their survival over time [57,58,59,60]. Biofilm formation, however, depends on several factors, including the physicochemical interactions between bacterial cells, the properties of the olive surface and the aqueous phase, the capability to produce EPS and the presence of specific regulatory genes [58,59,60].
Several authors demonstrated that table olives supported the formation of poly-microbial biofilms, including a cooperation between LAB (Lpb. plantarum [43,57,58] and Lpb. pentosus [43,60,61]) and yeasts (Candida famata, Candida ciferrii, Rhodotorula mucilaginosa, Crytococcus laurentii, Pichiaguillier mondii [58], Pichia galeiformis, Candida sorbosa, Geotrichum candidum [57,61] and Pichia membranifaciens [60]).
Kachouri et al. [58], using a scanning electron microscope, demonstrated the ability of Lpb. plantarum to adhere to olive surfaces during the storage of Chetoui table olives; the biofilm, moreover, promoted a reduction of undesirable microorganisms (moulds and yeasts already present on olive fruits) probably due to competition for nutrients and oxygen, the synthesis of antimicrobial products or modifications in the physicochemical properties of the olives.
The ability to adhere to olive surfaces may be also a survival strategy during transit into gastro-intestinal tract (GIT). Some Lactobacillus strains may have functions beneficial to the human host and, thus, the ability to cope with GIT conditions may be a convenient selection criterion.
In this study, the resistance to GIT-associated stresses was also evaluated. The % of log cycle reduction in simulated saliva (SS), gastric (SGJ) and pancreatic (SPJ) juices are shown in Figure 5. With the exception of Lpb. plantarum ISLCPT57, which was sensitive to simulated GIT transit (3.03 log cycle reduction), the other Lactiplantibacillus strains were quite tolerant, showing an overall decrease in survival ranging from 0.12 to 1.48 log cycles. As expected, SS conferred the least stress, while the effect of SGJ and SPJ was strain-dependent. Lpb. pentosus O17 was the most tolerant strain.
Arroyo-López et al. [62], using a TIM model to simulate gastric and intestinal human digestion, showed a considerable resistance of two olive-associated Lpb. pentosus strains to gastric digestion and the distal tract of the GIT (i.e., the jejunum and ileum). Botta et al. [63] demonstrated several potential probiotic features of Lpb. plantarum and Lpb. pentosus strains, including the resistance to simulated gastric digestion (human intestinal epithelial cell line model). These studies underline the possible use of fermented table olives as a functional food, being a promising vehicle to transfer microorganisms into the human body [5,62,63].
During the production of fermented olives, both natural microbiota and starter cultures must survive in the presence of the high salt concentrations and low pH values that characterize most fermentation brines [5,10].
In this study, the ability to grow at different combinations of NaCl concentrations and pH values was evaluated using a synthetic medium. The harshest combination (8% NaCl, pH 3.0) inhibited the growth of all strains after both 24 and 48 h of incubation (Figure 6). Overall, salt concentrations ≥ 6% NaCl significantly impaired strain cultivation, regardless of the pH conditions. Survival in less severe combinations (i.e., NaCl ≤ 6%; pH ≥ 4.0–4.5 commonly reached during olive fermentation), however, was also strain-specific.

3.4. Survival in Olive Mill Wastewater

As already mentioned, the resistance of Lactiplantibacillus to individual phenolic compounds has been reported for several strains [12], but the response to complex phenol-rich matrices (with the interaction of several components) has been scantly investigated. In this study, we used OMWs from Leccino, Coratina and Cima di Melfi cultivars as model substrates. OMW resulting from olive oil production, in fact, contains up to 80% of total phenols and fully reflects the phenolic profile of olive fruits.
In this study, no strain was able to survive in undiluted OMW, while tolerance to diluted OMWs (15 min incubation) depended on the cultivar (Table 2). Coratina affected strain survival to a greater extent, while Cima di Melfi provided the least stressful conditions. The most tolerant strains (Lpb. pentosus O17 and OM24 from olives, Lpb. plantarum C17 from cheese and Lpb. plantarum MTDA11S from sourdoughs) were further tested for OMW tolerance by using prolonged incubation times (Figure S2). The results confirmed that the Cima di Melfi OMW had the lowest inhibitory activity, while the survival in Coratina and Leccino OMWs depended on both strain and incubation time. Lpb. pentosus O17 exhibited the greatest robustness to OMWs, with all samples coping even for 30 min (albeit at very diluted concentrations).
To understand the possible factors affecting strain survival in OMWs, the total polyphenol content (TPC) and the phenolic profile were evaluated for all OMW samples. Cima di Melfi had the highest TPC (11.9 ± 0.3 g/kg) compared to the Coratina OMW (8.8 ± 0.2 g/kg) and Leccino (7.2 ± 0.3 g/kg) cultivars. Verbascoside, β-OH-verbascoside isomers and an oleuropein derivative were the main phenolic compounds of OMWs (Figure 7), although their occurrence was cultivar-dependent. Verbascoside was abundant in Coratina and Cima di Melfi samples, but was hardly present in the Leccino cultivar; β-OH-verbascoside, instead, was significantly present in Coratina and Leccino OMWs, but not in Cima di Melfi. An oleuropein derivative was common to all cultivars at comparable concentrations. The content of tyrosol and hydroxytyrosol was low in all samples. Overall, Coratina OMW had the highest amounts of all detected phenolic compounds and, most likely, this was correlated to its stronger inhibitory activity.
The antimicrobial activity of OMW and the synergistic effect of related phenolic compounds have been demonstrated by several authors. Tafesh et al. [64] found that some Gram+ (e.g., Streptococcus pyogenes and Staphylococcus aureus) and Gram− (e.g., Escherichia coli and Klebsiella pneumoniae) pathogens may be inhibited by using OMW extracts. Abu-Lafi et al. [65] also demonstrated that OMW extracts had an inhibitory activity against St. aureus and E. coli that was higher than that of antibiotics commonly used for their inactivation.
More recently, Belaqziz et al. [66] suggested that the antioxidant and antimicrobial activity (i.e., against Lactococcus lactis, Lactobacillus bulgaricus, St. aureus, Bacillus subtilis, L. innocua, Escherichia coli and Salmonella typhimurium) of OMW and table olive wastewaters (TOW) depended on both total phenolic content and the relative balance of phenolic compounds.
In this study, Lactiplantibacillus strains significantly suffered in OMW, and most of them survived when incubated in diluted samples (from 25% to 3.12%; from 4 to 32 dilutions of TPC of each cultivar). Previously, Ayed and Hamdi [67] demonstrated that Lpb. plantarum was able to survive in diluted OMW, removing 46% of total phenolic compounds; successively, Kachouri et al. [56] confirmed that undiluted OMW inhibited the growth of Lpb. plantarum, but in diluted samples, the strain led to degradation and removal (up to 63%) of several phenolic compounds (e.g., tyrosol, gallic, p-coumaric and caffeic acids).
In this study, the presence and interaction of verbascoside and β-OH-verbascoside isomers (found in Coratina cv.) mainly affected the strain survival. The high amounts of verbascoside and β-OH-verbascoside isomers in Coratina OMW was already demonstrated by Cardinali et al. [30] and D′Antuono et al. [68]; phenylpropanoid glycoside, however, was also found in OMW, resulting from different cultivars of Greek olives (e.g., Koroneiki and Lianiolia [68,69]).

3.5. Genome Sequencing of Lpb. pentosus O17 and Occurrence Analysis of Genes Involved in Degradation and Metabolism of Phenolic Compounds

The draft genome of Lpb. pentosus O17 (average coverage of 800.0×) contained 53 contigs, a circular chromosome of 3,850,701 bp and an overall GC content of 45.9%. A total of 3401 protein-coding sequences, 54 pseudogenes, 59 tRNA genes, 3 rRNA genes, 4 noncoding RNA (ncRNA) and 5 CRISPR arrays were identified.
The occurrence of the most important genes (β-glucosidase, gallate decarboxylase subunits B, C and D, p-coumaric acid decarboxylase, esterase, carboxylesterase, tannase subunits A and B and transcriptional regulator PadR) involved in the degradation and metabolism of phenolic compounds (Table S2; published data available for Lpb. plantarum and Lpb. pentosus strains) was verified in the genome of Lpb. pentosus O17.
The strain has an interesting gene pool and lacks only carboxylesterase and gallate decarboxylase subunits B and D. The gene profile of Lpb. pentosus O17 was compared with that of 28 (4 finished, 24 permanent draft) publicly available Lpb. pentosus genomes.
The genes of β-glucosidase, esterase, gallate decarboxylase (subunits B and C; lpdB and lpdC), p-coumaric acid decarboxylase (except for Lpb. pentosus 1.8.9), carboxylesterase and the transcriptional regulator PadR were present in all Lpb. pentosus genomes analysed (Table S5). On the contrary, the occurrence of gallate decarboxylase (subunit D; lpdD) and tannase (subunits A and B; tanA and tanB) sequences slightly differed among the analysed genomes; tanA and/or tanB occurred in most of them (93%), while lpdD was present only in Lpb. pentosus 3.2.8. Most of the strains were isolated from vegetable materials (i.e., corn silage, cucumber or olive fermentation and mustard pickles), while two strains were collected from human (vagina of a healthy Nigerian woman) and environmental (temperate deciduous forest biome soil) sources.
Most of the studies related to the genes involved in the metabolism of phenolic compounds focused on Lpb. plantarum species, although some data were also present for Lpb. paraplantarum and Lpb. pentosus species.
The metabolism of phenolic compounds is dynamic and quite complex. Besides the presence of genes, it is crucial to understand the interaction and regulation mechanisms of related degrading enzymes. Carrasco et al. [17] found that in some Lpb. pentosus strains, the exposure to different phenolic compounds (i.e., gallic, p-coumaric, caffeic, ferulic, vanillic, oleuropein, tyrosol, hydroxytyrosol and verbascoside) induced the concurrent over-expression of several genes (i.e., gallate decarboxylase, p-coumaric decarboxylase and tannase), suggesting that the degradation and metabolism of phenolic compounds may be related to the synergic effect of different degrading enzymes.
Landete et al. [12] reported that, in Lpb. plantarum, gallate decarboxylase may be involved in the decarboxylation of both gallic acid and protocatechuic acid, and tannase (a specific class of esterase) may also exert this function [70]. Actually, it was demonstrated that the sequential action of esterase and decarboxylases drives the proper degradation of hydroxybenzoic (tannase/gallate decarboxylase) and hydroxycinnamic (esterase/phenolic acid decarboxylase) acids [18]. Tannase was investigated in several strains of Lpb. plantarum but, to date, very few data [17,71] are available for Lpb. paraplantarum and Lpb. pentosus species. In this study, we found that tannase-encoding genes (mainly tanB) were widespread among Lpb. pentosus strains.
Although the β-glucosidase gene was present in all Lpb. pentosus genomes, phenotypic evidence demonstrated that its occurrence is not always related to oleuropein degradation [6,17] and, therefore, further studies are needed to correlate genetic information and strain metabolism.

4. Conclusions

A high level of diversity within the strains and species of the Lactiplantibacillus group was found in this study. In the screening step, the features that provided high variability among the strains were related to the capability to inhibit Yarrowia lipolytica, to produce EPS from glucose, maltose and sucrose, acid from xylose, hydroxytyrosol from oleuropein and to cope with gallic acid. On the contrary, most of strains tolerated protocatechuic and syringic acids, while hydroxybenzoic acid provided the highest level of toxicity.
Some selected strains were also able to produce biofilm, scavenge toxic radicals and survive the simulated GIT and simulated brine, suggesting their possible used as starter for the production of fermented table olives.
Moreover, although most of the strains had poor resistance to OMWs (used as a complex phenolic-rich matrix), our results provided progress in knowledge on the survival of the Lactiplantibacillus group to phenolic compounds. As the latter significantly differ (in terms of content and profile) among olive cultivars, the presence of proper degrading enzymes may be a helpful criterion for the selection of robust strains.
Additionally, the genome in silico analysis provided further information on the occurrence of genes involved in phenolic compound metabolism in Lpb. pentosus species, although the number of available genomes is significant lower compared to the closely related species Lpb. plantarum.
Contrary to some data available in the literature, in this study, some features related to the production of fermented olives (e.g., oleuropein degradation and hydroxytyrosol formation, tolerance to phenolic compounds and biofilm formation) were not strictly associated with isolation sources, and our data suggest that strains isolated from other sources (e.g., sourdoughs) can be also used as starter for the production of fermented table olives.
In this study, in fact, besides the olive-associated strain Lpb. pentosus O17, the Lpb. plantarum MT2A11S isolated from sourdoughs (both tolerant to phenolic compounds, able to produce biofilm and with high stress robustness) may also be used for the production of fermented olives.

Supplementary Materials

The following supporting information can be downloaded at: https://www.mdpi.com/article/10.3390/microorganisms10030625/s1, Table S1: Reaction mixture and PCR program for the amplification of partial 16S rRNA genes; Table S2: List of genes involved in phenolic compound metabolism, used to verify the occurrence in publicly available genomes of Lactiplantibacillus paraplantarum, Lpb. plantarum and Lpb. pentosus (References [72,73,74,75] are cited in the Table S2); Table S3: Exopolysaccharide (EPS) production and antimicrobial activity of strains; Figure S1: Thin layer chromatography (TLC) of MRS samples unsupplemented and supplemented with oleuropein and hydroxytyrosol; Table S4: Qualitative evaluation of oleuropein degradation and hydroxytyrosol formation using thin layer chromatography (TLC); Figure S2: Resistance of Lpb. pentosus O17, OM24 and Lpb. plantarum C17, MT2A11S to different concentrations (from 50% to 6.12% v/v) of Leccino, Coratina and Cima di Melfi OMWs after 15, 30, 60 and 120 min of incubation at 30 °C; Table S5: Occurrence analysis of genes involved in degradation and metabolism of phenolic compounds in Lactiplantibacillus pentosus genomes.

Author Contributions

Conceptualization, E.P., T.Z. and A.R.; methodology, T.Z., A.R. and G.P.; formal analysis, M.G., G.P. and F.S.; investigation, M.G., G.P. and F.S.; data curation, E.P. and T.Z.; writing—original draft preparation, E.P. and T.Z; writing—review and editing, E.P., T.Z., A.R., M.G. and G.P.; supervision, E.P., T.Z. and A.R. All authors have read and agreed to the published version of the manuscript.

Funding

This work was partially funded by Ministero delle Politiche Agricole, Alimentari e Forestali (MIPAAF), Rome, Italy; Project IT4NUEVOO (ID-15; Ministerial Decree n. 30311 del 31/10/2018).

Data Availability Statement

Not applicable.

Acknowledgments

We thank Maria Aponte, Università degli Studi di Napoli Federico II, for providing the strains Lactiplantibacillus pentosus OM24, OM53, OM52, OM62, OM50, OM13, OM14 and OM35.

Conflicts of Interest

The authors declare no conflict of interest.

References

  1. Zheng, J.; Wittouck, S.; Salvetti, E.; Franz, C.M.A.P.; Harris, H.M.B.; Mattarelli, P.; O’Toole, P.W.; Pot, B.; Vandamme, P.; Walter, J.; et al. A taxonomic note on the genus Lactobacillus: Description of 23 novel genera, emended description of the genus Lactobacillus Beijerinck 1901, and union of Lactobacillaceae and Leuconostocaceae. Int. J. Syst. Evol. Microbiol. 2020, 70, 2782–2858. [Google Scholar] [CrossRef] [PubMed]
  2. Martino, M.E.; Bayjanov, J.R.; Caffrey, B.E.; Wels, M.; Joncour, P.; Hughes, S.; Gillet, B.; Kleerebezem, M.; van Hijum, S.A.; Leulier, F. Nomadic lifestyle of Lactobacillus plantarum revealed by comparative genomics of 54 strains isolated from different habitats. Environ. Microbiol. 2016, 18, 4974–4989. [Google Scholar] [CrossRef] [PubMed]
  3. Cen, S.; Yin, R.; Mao, B.; Zhao, J.; Zhang, H.; Zhai, Q.; Chen, W. Comparative genomics shows niche-specific variations of Lactobacillus plantarum strains isolated from human, Drosophila melanogaster, vegetable and dairy sources. Food Biosci. 2020, 35, 100581. [Google Scholar] [CrossRef]
  4. Mao, B.; Yin, R.; Li, X.; Cui, S.; Zhang, H.; Zhao, J.; Chen, W. Comparative genomic analysis of Lactiplantibacillus plantarum isolated from different niches. Genes 2021, 12, 241. [Google Scholar] [CrossRef]
  5. Perpetuini, G.; Prete, R.; Garcia-Gonzalez, N.; Alam, M.K.; Corsetti, A. Table olives more than a fermented food. Foods 2020, 9, 178. [Google Scholar] [CrossRef] [Green Version]
  6. Vaccalluzzo, A.; Pino, A.; Russo, N.; De Angelis, M.; Caggia, C.; Randazzo, C.L. FoodOmics as a new frontier to reveal microbial community and metabolic processes occurring on table olives fermentation. Food Microbiol. 2020, 92, 103606. [Google Scholar] [CrossRef]
  7. Servili, M.; Settanni, L.; Veneziani, G.; Esposto, S.; Massitti, O.; Taticchi, A.; Urbani, S.; Montedoro, G.F.; Corsetti, A. The use of Lactobacillus pentosus 1MO to shorten the debittering process time of black table olives (Cv. Itrana and Leccino): A pilot-scale application. J. Agric. Food Chem. 2006, 54, 3869–3875. [Google Scholar] [CrossRef]
  8. Bleve, G.; Tufariello, M.; Durante, M.; Perbellini, E.; Ramires, F.A.; Grieco, F.; Cappello, M.S.; De Domenico, M.; Mita, M.; Tasioula-Margari, M.; et al. Physico-chemical and microbiological characterization of spontaneous fermentation of Cellina di Nardò and Leccino table olives. Front. Microbiol. 2014, 5, 570. [Google Scholar] [CrossRef] [Green Version]
  9. Tofalo, R.; Perpetuini, G.; Schirone, M.; Ciarrocchi, A.; Fasoli, G.; Suzzi, G.; Corsetti, A. Lactobacillus pentosus dominates spontaneous fermentation of Italian table olives. LWT-Food Sci. Technol. 2014, 57, 710–717. [Google Scholar] [CrossRef]
  10. Corsetti, A.; Perpetuini, G.; Schirone, M.; Tofalo, R.; Suzzi, G. Application of starter cultures to table olive fermentation: An overview on the experimental studies. Front. Microbiol. 2012, 3, 248. [Google Scholar] [CrossRef] [Green Version]
  11. Hurtado, A.; Reguant, C.; Bordons, A.; Rozès, N. Lactic acid bacteria from fermented table olives. Food Microbiol. 2012, 31, 1–8. [Google Scholar] [CrossRef] [PubMed]
  12. Landete, J.M.; Rodriguez, H.; Curiel, J.A.; de las Rivas, B.; López de Felipe, F.; Muñoz, R. Degradation of phenolic compounds found in olive products by Lactobacillus plantarum strains. In Olives and Olive Oil in Health and Disease Prevention, 2nd ed.; Preedy, V.R., Watson, R.R., Eds.; Elsevier, Academic Press: Amsterdam, The Netherlands, 2021; pp. 133–144. [Google Scholar] [CrossRef]
  13. Perpetuini, G.; Scornec, H.; Tofalo, R.; Serror, P.; Schirone, M.; Suzzi, G.; Corsetti, A.; Cavin, J.F.; Licantro-Seraut, H. Identification of critical genes for growth in olive brine by transposon mutagenesis of Lactobacillus pentosus C11. Appl. Environ. Microbiol. 2013, 79, 4568–4575. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  14. Esteban-Torres, M.; Reverón, I.; Mancheño, J.M.; de las Rivas, B.; Muñoz, R. Characterization of a Feruloyl Esterase from Lactobacillus plantarum. Appl. Environ. Microbiol. 2013, 79, 5130–5136. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  15. Jiménez, N.; Curiel, J.A.; Reverón, I.; de las Rivas, B.; Muñoz, R. Uncovering the Lactobacillus plantarum WCFS1 Gallate Decarboxylase Involved in Tannin Degradation. Appl. Environ. Microbiol. 2013, 79, 4253–4263. [Google Scholar] [CrossRef] [Green Version]
  16. Reverón, I.; Jiménez, N.; Curiel, J.A.; Peñas, E.; López de Felipe, F.; de las Rivas, B.; Muñoz, R. Differential gene expression by Lactobacillus plantarum WCFS1 in response to phenolic compounds reveals new genes involved in tannin degradation. Appl. Environ. Microbiol. 2017, 83, e03387-16. [Google Scholar] [CrossRef] [Green Version]
  17. Carrasco, J.A.; Lucena-Padrós, H.; Brenes, M.; Ruiz-Barba, J.L. Expression of genes involved in metabolism of phenolic compounds by Lactobacillus pentosus and its relevance for table-olive fermentations. Food Microbiol. 2018, 76, 382–389. [Google Scholar] [CrossRef] [Green Version]
  18. Landete, J.M.; Plaza-Vinuesa, L.; Montenegro, C.; Santamaría, L.; Reverón, I.; de las Rivas, B.; Muñoz, R. The use of Lactobacillus plantarum esterase genes: A biotechnological strategy to increase the bioavailability of dietary phenolic compounds in lactic acid bacteria. Int. J. Food Sci. Nutr. 2021, 72, 1035–1045. [Google Scholar] [CrossRef]
  19. Zotta, T.; Ricciardi, A.; Guidone, A.; Sacco, M.; Muscariello, L.; Mazzeo, M.F.; Cacace, G.; Parente, E. Inactivation of ccpA and aeration affect growth, metabolite production and stress tolerance Lactobacillus plantarum WCFS1. Int. J. Food Microbiol. 2012, 155, 51–59. [Google Scholar] [CrossRef]
  20. Ricciardi, A.; Parente, E.; Tramutola, T.; Guidone, A.; Ianniello, R.G.; Pavlidis, D.; Tsakalidou, E.; Zotta, T. Evaluation of a differential medium for the preliminary identification of members of the Lactobacillus plantarum and Lactobacillus casei groups. Ann. Microbiol. 2015, 65, 1649–1658. [Google Scholar] [CrossRef]
  21. Parente, E.; Ciocia, F.; Ricciardi, A.; Zotta, T.; Felis, G.E.; Torriani, S. Diversity of stress tolerance in Lactobacillus plantarum, Lactobacillus pentosus and Lactobacillus paraplantarum: A multivariate screening study. Int. J. Food Microbiol. 2010, 144, 270–279. [Google Scholar] [CrossRef]
  22. Torriani, S.; Felis, G.E.; Dellaglio, F. Differentiation of Lactobacillus plantarum, L. pentosus, and L. paraplantarum by recA gene sequence analysis and multiplex PCR assay with recA gene-derived primers. Appl. Environ. Microbiol. 2001, 67, 3450–3454. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  23. Parente, E.; Grieco, S.; Crudele, M.A. Phenotypic diversity of lactic acid bacteria isolated from fermented sausages produced in Basilicata (Southern Italy). J. Appl. Microbiol. 2001, 90, 943–952. [Google Scholar] [CrossRef] [PubMed]
  24. Zotta, T.; Ricciardi, A.; Ianniello, R.G.; Parente, E.; Reale, A.; Rossi, F.; Iacumin, L.; Comi, G.; Coppola, R. Assessment of aerobic and respiratory growth in the Lactobacillus casei group. PLoS ONE 2014, 9, e99189. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  25. Ciafardini, G.; Marsilio, V.; Lanza, B.; Pozzi, N. Hydrolysis of oleuropein by Lactobacillus plantarum strains associated with olive fermentation. Appl. Environ. Microbiol. 1994, 60, 4142–4147. [Google Scholar] [CrossRef] [Green Version]
  26. Wang, A.N.; Yi, X.W.; Yu, H.F.; Dong, B.; Qiao, S.Y. Free radical scavenging activity of Lactobacillus fermentum in vitro and its antioxidative effect on growing-finishing pigs. J. Appl. Microbiol. 2009, 107, 1140–1148. [Google Scholar] [CrossRef]
  27. Guidone, A.; Zotta, T.; Ross, R.P.; Stanton, C.; Rea, M.C.; Parente, E.; Ricciardi, A. Functional properties of Lactobacillus plantarum strains: A multivariate screening study. LWT-Food Sci. Technol. 2014, 56, 69–76. [Google Scholar] [CrossRef]
  28. Ricciardi, A.; Guidone, A.; Ianniello, R.G.; Cioffi, S.; Aponte, M.; Pavlidis, D.; Tsakalidou, E.; Zotta, T.; Parente, E. A survey of non-starter lactic acid bacteria in traditional cheeses: Culture dependent identification and survival to simulated gastrointestinal transit. Int. Dairy J. 2015, 43, 42–50. [Google Scholar] [CrossRef]
  29. Ianniello, R.G.; Ricciardi, A.; Parente, E.; Tramutola, A.; Reale, A.; Zotta, T. Aeration and supplementation with heme and menaquinone affect survival to stresses and antioxidant capability of Lactobacillus casei strains. LWT-Food Sci. Technol. 2015, 60, 817–824. [Google Scholar] [CrossRef]
  30. Cardinali, A.; Pati, S.; Minervini, F.; D’Antuono, I.; Linsalata, V.; Lattanzio, V. Verbascoside, isoverbascoside, and their derivatives recovered from olive mill wastewater as possible food antioxidants. J. Agric. Food Chem. 2012, 60, 1822–1829. [Google Scholar] [CrossRef]
  31. R Core Team. R: A Language and Environment for Statistical Computing; R Foundation for Statistical Computing: Vienna, Austria, 2021; Available online: https://www.R-project.org (accessed on 15 January 2022).
  32. Ribeiro, T.B.; Oliveira, A.L.; Costa, C.; Nunes, J.; Vicente, A.A.; Pintado, M. Total and sustainable valorisation of olive pomace using a fractionation approach. Appl. Sci. 2020, 10, 6785. [Google Scholar] [CrossRef]
  33. Pot, B.; Felis, G.E.; De Bruyne, K.; Tsakalidou, E.; Papadimitriou, K.; Leisner, J.; Vanadmme, P. The genus Lactobacillus. In Lactic Acid Bacteria: Biodiversity and Taxonomy; Hlzapfel, W.H., Wood, B.J.B., Eds.; John Wiley & Sons: Hoboken, NJ, USA, 2014; pp. 249–353. [Google Scholar] [CrossRef]
  34. Marsilio, V.; Lanza, B. Characterisation of an oleuropein degrading strain of Lactobacillus plantarum. Combined effects of compounds present in olive fermenting brines (phenols, glucose and NaCl) on bacterial activity. J. Sci. Food Agric. 1998, 76, 520–524. [Google Scholar] [CrossRef]
  35. Iorizzo, M.; Lombardi, S.J.; Macciola, V.; Testa, B.; Lustrato, G.; Lopez, F.; De Leonardis, A. Technological potential of Lactobacillus strains isolated from fermented green olives: In vitro studies with emphasis on oleuropein-degrading capability. Sci. World J. 2016, 2016, 1917592. [Google Scholar] [CrossRef] [Green Version]
  36. Zago, M.; Lanza, B.; Rossetti, L.; Muzzalupo, I.; Carminati, D.; Giraffa, G. Selection of Lactobacillus plantarum strains to use as starters in fermented table olives: Oleuropeinase activity and phage sensitivity. Food Microbiol. 2013, 34, 81–87. [Google Scholar] [CrossRef] [PubMed]
  37. Bautista-Gallego, J.; Arroyo-López, F.N.; Romero-Gil, V.; Rodríguez-Gómez, F.; García-García, P.; Garrido-Fernández, A. Fermentation profile of green Spanish-style Manzanilla olives according to NaCl content in brine. Food Microbiol. 2015, 49, 56–64. [Google Scholar] [CrossRef] [PubMed]
  38. Pino, A.; De Angelis, M.; Todaro, A.; Van Hoorde, K.; Randazzo, C.L.; Caggia, C. Fermentation of Nocellara Etnea table olives by functional starter cultures at different low salt concentrations. Front. Microbiol. 2018, 9, 1125. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  39. Caggianiello, G.; Kleerebezem, M.; Spano, G. Exopolysaccharides produced by lactic acid bacteria: From health-promoting benefits to stress tolerance mechanisms. Appl. Microbiol. Biotechnol. 2016, 100, 3877–3886. [Google Scholar] [CrossRef]
  40. Arroyo-López, F.N.; Querol, A.; Bautista-Gallego, J.; Garrido-Fernández, A. Role of yeasts in table olive production. Int. J. Food Microbiol. 2008, 128, 189–196. [Google Scholar] [CrossRef] [PubMed]
  41. Caggia, C.; Randazzo, C.L.; Di Salvo, M.; Romeo, F.; Giudici, P. Association for food protection occurrence of Listeria monocytogenes in green table olives. J. Food Prot. 2004, 67, 2189–2194. [Google Scholar] [CrossRef] [PubMed]
  42. Bevilacqua, A.; Campaniello, D.; Speranza, B.; Sinigaglia, M.; Corbo, M.R. Survival of Listeria monocytogenes and Staphylococcus aureus in synthetic brines. studying the effects of salt, temperature and sugar through the approach of the design of experiments. Front. Microbiol. 2018, 9, 240. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  43. Benítez-Cabello, A.; Calero-Delgado, B.; Rodríguez-Gómez, F.; Garrido-Fernández, A.; Jiménez-Díaz, R.; Arroyo-López, F.N. Biodiversity and multifunctional features of lactic acid bacteria isolated from table olive biofilms. Front. Microbiol. 2019, 10, 836. [Google Scholar] [CrossRef]
  44. Abouloifa, H.; Gaamouche, S.; Rokni, Y.; Hasnaoui, I.; Bellaouchi, R.; Ghabbour, N.; Karboune, S.; Brasca, M.; D’Hallewin, G.; Ben Salah, R.; et al. Antifungal activity of probiotic Lactobacillus strains isolated from natural fermented green olives and their application as food bio-preservative. Biol. Control 2021, 152, 104450. [Google Scholar] [CrossRef]
  45. Johnson, R.L.; Mitchell, A.E. Reducing phenolics related to bitterness in table olives. J. Food Qual. 2018, 2018, 3193185. [Google Scholar] [CrossRef]
  46. Santos, M.M.; Piccirillo, C.; Castro, P.M.L.; Kalogerakis, N.; Pintado, M.E. Bioconversion of oleuropein to hydroxytyrosol by lactic acid bacteria. World J. Microbiol. Biotechnol. 2012, 28, 2435–2440. [Google Scholar] [CrossRef] [PubMed]
  47. Kaltsa, A.; Papaliaga, D.; Papaioannou, E.; Kotzekidou, P. Characteristics of oleuropeinolytic strains of Lactobacillus plantarum group and influence on phenolic compounds in table olives elaborated under reduced salt conditions. Food Microbiol. 2015, 48, 58–62. [Google Scholar] [CrossRef] [PubMed]
  48. Ramírez, E.; Brenes, M.; de Castro, A.; Romero, C.; Medina, E. Oleuropein hydrolysis by lactic acid bacteria in natural green olives. LWT-Food Sci. Technol. 2017, 78, 165–171. [Google Scholar] [CrossRef]
  49. Petridis, A.; Therios, I.; Samouris, G. Genotypic variation of total phenol and oleuropein concentration and antioxidant activity of 11 Greek olive cultivars (Olea europaea L.). HortScience 2012, 47, 339–342. [Google Scholar] [CrossRef] [Green Version]
  50. Santamaría, L.; Reverón, I.; Plaza-Vinuesa, L.; Oliveros, J.C.; de las Rivas, B.; Muñoz, R.; López de Felipe, F. Oleuropein transcriptionally primes Lactobacillus plantarum to interact with plant hosts. Front. Microbiol. 2019, 10, 2177. [Google Scholar] [CrossRef]
  51. Karković Marković, A.; Torić, J.; Barbarić, M.; Jakobušić Brala, C. Hydroxytyrosol, tyrosol and derivatives and their potential effects on human health. Molecules 2019, 24, 2001. [Google Scholar] [CrossRef] [Green Version]
  52. Bertelli, M.; Kiani, A.K.; Paolacci, S.; Manara, E.; Kurti, D.; Dhuli, K.; Bushati, V.; Miertus, J.; Pangallo, D.; Baglivo, M.; et al. Hydroxytyrosol: A natural compound with promising pharmacological activities. J. Biotechnol. 2019, 309, 29–33. [Google Scholar] [CrossRef]
  53. Kachouri, F.; Ksontini, H.; Kraiem, M.; Setti, K.; Mechmeche, M.; Hamdi, M. Involvement of antioxidant activity of Lactobacillus plantarum on functional properties of olive phenolic compounds. J. Food Sci. Technol. 2015, 52, 7924–7933. [Google Scholar] [CrossRef] [Green Version]
  54. Kachouri, F.; Hamdi, M. Use Lactobacillus plantarum in olive oil process and improvement of phenolic compounds content. J. Food Eng. 2006, 77, 746–752. [Google Scholar] [CrossRef]
  55. Hamid abadi Sherahi, M.; Shahidi, F.; Yazdi, F.T.; Hashemi, S.M.B. Effect of Lactobacillus plantarum on olive and olive oil quality during fermentation process. LWT-Food Sci. Technol. 2018, 89, 572–580. [Google Scholar] [CrossRef]
  56. Kachouri, F.; Setti, K.; Ksontini, H.; Mechmeche, M.; Hamdi, M. Improvement of antioxidant activity of olive mill wastewater phenolic compounds by Lactobacillus plantarum fermentation. Desalin. Water Treat. 2016, 57, 27125–27137. [Google Scholar] [CrossRef]
  57. Domínguez-Manzano, J.; León-Romero, Á.; Olmo-Ruiz, C.; Bautista-Gallego, J.; Arroyo-López, F.N.; Garrido-Fernández, A.; Jiménez-Díaz, R. Biofilm formation on abiotic and biotic surfaces during Spanish style green table olive fermentation. Int. J. Food Microbiol. 2012, 157, 230–238. [Google Scholar] [CrossRef]
  58. Kachouri, F.; Hamida, K.; Soumya El, A.; Saad, I.S.; Hasna, M.; Hassan, L.; Moktar, H. Lactobacillus plantarum: Effect of a protective biofilm on the surface of olives during storage. Braz. J. Microbiol. 2016, 47, 202–209. [Google Scholar] [CrossRef] [Green Version]
  59. Perpetuini, G.; Pham-Hoang, B.N.; Scornec, H.; Tofalo, R.; Schirone, M.; Suzzi, G.; Cavin, J.F.; Waché, Y.; Corsetti, A.; Licandro-Seraut, H. In Lactobacillus pentosus, the olive brine adaptation genes are required for biofilm formation. Int. J. Food Microbiol. 2016, 216, 104–109. [Google Scholar] [CrossRef]
  60. Benítez-Cabello, A.; Romero-Gil, V.; Rodríguez-Gómez, F.; Garrido-Fernández, A.; Jiménez-Díaz, R.; Arroyo-López, F.N. Evaluation and identification of poly-microbial biofilms on natural green Gordal table olives. Antonie Van Leeuwenhoek 2015, 108, 597–610. [Google Scholar] [CrossRef] [Green Version]
  61. Arroyo-López, F.N.; Bautista-Gallego, J.; Domínguez-Manzano, J.; Romero-Gil, V.; Rodriguez-Gómez, F.; García-García, P.; Garrido-Fernández, A.; Jiménez-Díaz, R. Formation of lactic acid bacteria–yeasts communities on the olive surface during Spanish-style Manzanilla fermentations. Food Microbiol. 2012, 32, 295–301. [Google Scholar] [CrossRef]
  62. Arroyo-López, F.N.; Blanquet-Diot, S.; Denis, S.; Thévenot, J.; Chalancon, S.; Alric, M.; Rodríguez-Gómez, F.; Romero-Gil, V.; Jiménez-Díaz, R.; Garrido-Fernández, A. Survival of pathogenic and lactobacilli species of fermented olives during simulated human digestion. Front. Microbiol. 2014, 5, 540. [Google Scholar] [CrossRef]
  63. Botta, C.; Langerholc, T.; Cencič, A.; Cocolin, L. In vitro selection and characterization of new probiotic candidates from table olive microbiota. PLoS ONE 2014, 9, e94457. [Google Scholar] [CrossRef]
  64. Tafesh, A.; Najami, N.; Jadoun, J.; Halahlih, F.; Riepl, H.; Azaizeh, H. Synergistic antibacterial effects of polyphenolic compounds from olive mill wastewater. Evid.-Based Complement. Altern. Med. 2011, 2011, 431021. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  65. Abu-Lafi, S.; Al-Natsheh, M.S.; Yaghmoor, R.; Al-Rimawi, F. Enrichment of phenolic compounds from olive mill wastewater and in vitro evaluation of their antimicrobial activities. Evid.-Based Complement. Altern. Med. 2017, 2017, 3706915. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  66. Belaqziz, M.; Tan, S.P.; El-Abbassi, A.; Kiai, H.; Hafidi, A.; O’Donovan, O.; McLoughlin, P. Assessment of the antioxidant and antibacterial activities of different olive processing wastewaters. PLoS ONE 2017, 12, e0182622. [Google Scholar] [CrossRef] [PubMed]
  67. Ayed, L.; Hamdi, M. Fermentative decolorization of olive mill wastewater by Lactobacillus plantarum. Process. Biochem. 2003, 39, 59–65. [Google Scholar] [CrossRef]
  68. D’Antuono, I.; Kontogianni, V.G.; Kotsiou, K.; Linsalata, V.; Logrieco, A.F.; Tasioula-Margari, M.; Cardinali, A. Polyphenolic characterization of olive mill wastewaters, coming from Italian and Greek olive cultivars, after membrane technology. Food Res. Int. 2014, 65, 301–310. [Google Scholar] [CrossRef]
  69. Kanakis, P.; Termentzi, A.; Michel, T.; Gikas, E.; Halabalaki, M.; Skaltsounis, A.L. From olive drupes to olive oil. An HPLC-orbitrap-based qualitative and quantitative exploration of olive key metabolites. Planta Med. 2013, 79, 1576–1587. [Google Scholar] [CrossRef] [Green Version]
  70. Curiel, J.A.; Rodríguez, H.; Acebrón, I.; Mancheño, J.M.; De Las Rivas, B.; Muñoz, R. Production and physicochemical properties of recombinant Lactobacillus plantarum tannase. J. Agric. Food Chem. 2009, 57, 6224–6230. [Google Scholar] [CrossRef] [Green Version]
  71. Ueda, S.; Nomoto, R.; Yoshida, K.; Osawa, R. Comparison of three tannases cloned from closely related Lactobacillus species: L. plantarum, L. paraplantarum, and L. pentosus. BMC Microbiol. 2014, 14, 87. [Google Scholar] [CrossRef] [Green Version]
  72. Rodriguez, H.; Landete, J.M.; Curiel, J.A.; de las Rivas, B.; Mancheño, J.M.; Muñoz, R. Characterization of the p-Coumaric acid decarboxylase from Lactobacillus plantarum CECT 748T. J. Agric. Food Chem. 2008, 56, 3068–3072. [Google Scholar] [CrossRef]
  73. Jiménez, N.; Esteban-Torres, M.; Mancheño, J.M.; de las Rivas, B.; Muñoz, R. Tannin degradation by a novel tannase enzyme present in some Lactobacillus plantarum strains. Appl. Environ. Microbiol. 2014, 80, 2991–2997. [Google Scholar] [CrossRef] [Green Version]
  74. Pan, H.; Zhan, J.; Yang, H.; Wang, C.; Liu, H.; Zhou, H.; Zhou, H.; Lu, X.; Su, X.; Tian, Y. Improving the acid resistance of tannase TanBLp (AB379685) from Lactobacillus plantarum ATCC14917T by Site-Specific Mutagenesis. Indian J. Microbiol. 2021, 62, 96–102. [Google Scholar] [CrossRef]
  75. Esteban-Torres, M.; Landete, J.M.; Reverón, I.; Santamaría, L.; de las Rivas, B.; Muñoz, R. A Lactobacillus plantarum esterase active on a broad range of phenolic esters. Appl. Environ. Microbiol. 2015, 81, 3235–3242. [Google Scholar] [CrossRef] [Green Version]
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Figure 1. Correlation among technological properties of Lactiplantibacillus strains. Red box: positive; yellow box: negative. Code of columns of the dendrogram: YL, antimicrobial activity against Yarrowia lipolytica; M-MRS, S-MRS and G-MRS, production of exopolysaccharides on maltose, sucrose and glucose, respectively; Gall_100 (100 mM gallic acid), Pro_50 (50 mM protocatechuic acid), Hdb_20 (20 mM 4-hydroxybenzoic acid) and Srn_25 (25 mM syringic acid) referred to phenolic compound tolerance; xyl_cre, growth on xylose; xyl_ac, acid production from xylose; NaCl7_5, salt tolerance; CAT_heme, catalase activity; Ole_deg, oleuropein hydrolysis; Htyr, hydroxytyrosol formation. Rows of the dendrogram (similarity relationships among strains): LAB species: Lpl, Lpb. plantarum, Lpa, Lpb. paraplantarum, Lpe, Lpb. pentosus; isolation source: vegetables (violet), sourdoughs (blue), olives and derived products (yellow), dairy products (red), wine (orange), human sources (green), meat products (brown), unknown sources (pink).
Figure 1. Correlation among technological properties of Lactiplantibacillus strains. Red box: positive; yellow box: negative. Code of columns of the dendrogram: YL, antimicrobial activity against Yarrowia lipolytica; M-MRS, S-MRS and G-MRS, production of exopolysaccharides on maltose, sucrose and glucose, respectively; Gall_100 (100 mM gallic acid), Pro_50 (50 mM protocatechuic acid), Hdb_20 (20 mM 4-hydroxybenzoic acid) and Srn_25 (25 mM syringic acid) referred to phenolic compound tolerance; xyl_cre, growth on xylose; xyl_ac, acid production from xylose; NaCl7_5, salt tolerance; CAT_heme, catalase activity; Ole_deg, oleuropein hydrolysis; Htyr, hydroxytyrosol formation. Rows of the dendrogram (similarity relationships among strains): LAB species: Lpl, Lpb. plantarum, Lpa, Lpb. paraplantarum, Lpe, Lpb. pentosus; isolation source: vegetables (violet), sourdoughs (blue), olives and derived products (yellow), dairy products (red), wine (orange), human sources (green), meat products (brown), unknown sources (pink).
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Figure 2. Minimum inhibitory concentration (MIC, mg/L) of 4-hydroxybenzoic (Hdb, 40–2.5 mM), syringic (Srn, 25–1.56 mM), gallic (Gal, 100–6.25 mM) and protocatechuic (Pro, 50–3.12 mM) acids. Phenolic compound concentration is defined by different colours shades, from yellow (0 mg/L) to red (100 mg/L). Rows of the dendrogram: LAB species: Lpl, Lpb. plantarum, Lpa, Lpb. paraplantarum, Lpe, Lpb. pentosus; isolation source: vegetables (violet), sourdoughs (blue), olives and derived products (yellow), dairy products (red), wine (orange), human sources (green), meat products (brown), unknown sources (pink). Rows of the dendrogram show similarity relationships between strains based on phenolic compounds tolerance. Columns of the dendrogram show the similarity among the effect of phenolic compounds on Lactiplantibacillus strains.
Figure 2. Minimum inhibitory concentration (MIC, mg/L) of 4-hydroxybenzoic (Hdb, 40–2.5 mM), syringic (Srn, 25–1.56 mM), gallic (Gal, 100–6.25 mM) and protocatechuic (Pro, 50–3.12 mM) acids. Phenolic compound concentration is defined by different colours shades, from yellow (0 mg/L) to red (100 mg/L). Rows of the dendrogram: LAB species: Lpl, Lpb. plantarum, Lpa, Lpb. paraplantarum, Lpe, Lpb. pentosus; isolation source: vegetables (violet), sourdoughs (blue), olives and derived products (yellow), dairy products (red), wine (orange), human sources (green), meat products (brown), unknown sources (pink). Rows of the dendrogram show similarity relationships between strains based on phenolic compounds tolerance. Columns of the dendrogram show the similarity among the effect of phenolic compounds on Lactiplantibacillus strains.
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Figure 3. DPPH and hydroxyl radical scavenging activities in the 15 selected Lactiplantibacillus strains. Letters on plot bars indicate significant differences (Tukey′s HSD, p < 0.01) in scavenging activity within strains.
Figure 3. DPPH and hydroxyl radical scavenging activities in the 15 selected Lactiplantibacillus strains. Letters on plot bars indicate significant differences (Tukey′s HSD, p < 0.01) in scavenging activity within strains.
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Figure 4. Biofilm formation in the 15 selected Lactiplantibacillus strains after 24 and 48 h incubation. Colour: green Lpb. pentosus strains (isolated from olive and brine); blue, Lpb. plantarum strains (isolated from other sources, e.g., sourdoughs, cheese, human).
Figure 4. Biofilm formation in the 15 selected Lactiplantibacillus strains after 24 and 48 h incubation. Colour: green Lpb. pentosus strains (isolated from olive and brine); blue, Lpb. plantarum strains (isolated from other sources, e.g., sourdoughs, cheese, human).
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Figure 5. Percentage (%) of log cycle reduction measured at each step (numbers within bars) of simulated gastro-intestinal (GIT) transit (simulated saliva, SS; simulated gastric juice, SGJ; simulated pancreatic juice, SPJ). For each strain, survival was calculated as a reduction of log(N/N0), where N0 and N are the number of cells before and after exposure to each stress. The numbers in brackets, over the bars, indicate the overall log cycle reduction after all steps (complete simulated GIT transit).
Figure 5. Percentage (%) of log cycle reduction measured at each step (numbers within bars) of simulated gastro-intestinal (GIT) transit (simulated saliva, SS; simulated gastric juice, SGJ; simulated pancreatic juice, SPJ). For each strain, survival was calculated as a reduction of log(N/N0), where N0 and N are the number of cells before and after exposure to each stress. The numbers in brackets, over the bars, indicate the overall log cycle reduction after all steps (complete simulated GIT transit).
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Figure 6. Inhibition curves in response to NaCl concentrations (blue, 8% NaCl; green, 6% NaCl; red, 4% NaCl; orange, 0% NaCl) and pH values (x-axis), after 24 h (continuous lines) and 48 h (dotted lines) of incubation. Inhibition was calculated as (I0-I)/I0, where I0 was the response of the control (i.e., A650 at 0% NaCl and pH 6.0) and I is the response at any given concentration of salt and pH value.
Figure 6. Inhibition curves in response to NaCl concentrations (blue, 8% NaCl; green, 6% NaCl; red, 4% NaCl; orange, 0% NaCl) and pH values (x-axis), after 24 h (continuous lines) and 48 h (dotted lines) of incubation. Inhibition was calculated as (I0-I)/I0, where I0 was the response of the control (i.e., A650 at 0% NaCl and pH 6.0) and I is the response at any given concentration of salt and pH value.
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Figure 7. Phenolic profiles (HPLC chromatograms) of olive mill wastewater (OMW) resulting from olive oil production of Leccino, Coratina and Cima di Melfi cultivars. Peaks have been putatively assigned on the basis of retention time values (min) and by comparing them with literature data and UV spectra (280 nm).
Figure 7. Phenolic profiles (HPLC chromatograms) of olive mill wastewater (OMW) resulting from olive oil production of Leccino, Coratina and Cima di Melfi cultivars. Peaks have been putatively assigned on the basis of retention time values (min) and by comparing them with literature data and UV spectra (280 nm).
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Table
Table 1. List of Lactiplantibacillus strains used in this study.
Table 1. List of Lactiplantibacillus strains used in this study.
Source GroupSourceStrains and Species
Cheese (CH)Caciocavallo cheeseLpb. paraplantarum F10, B7N26; Lpb. plantarum B7N23; Lpb. plantarum subsp. plantarum B15, C17, S12
CheeseLpb. plantarum ISLCPT68; Lpb. plantarum subsp. argentoratensis FSL170; Lpb. plantarum subsp. plantarum ISLCPT57, FSM17
Meat product (M)SalamiLpb. pentosus LPL
Plant material (P)VegetablesLpb. plantarum subsp. plantarum S85, LM3
SilageLpb. plantarum subsp. plantarum DCU101, NCFB340
Olives (O)Olive brineLpb. pentosus 2TP, 4TP, 4TG, 5TP, P13.3; Lpb. plantarum subsp. plantarum P1.5
Treated table olives (Cerignola cv.)Lpb. pentosus O5 *; Lpb. plantarum: O1 *, O4 *
Natural table olives (Cerignola cv.)Lpb. pentosus O11 *, O12 *, O15 *; Lpb. plantarum O13*
Brine from treated table olives (Cerignola cv.)Lpb. pentosus O17 *, O18 *, O19 *, O20 *
Brine from natural table olives (Cerignola cv.) Lpb. pentosus O24 *
Table olives (Nocellara del Belice cv.)Lpb. pentosus OM24, OM53, OM52, OM62, OM50, OM13, OM14, OM35 #
Sourdough (SD)ManiocaLpb. plantarum subsp. plantarum DKO22, 38AA
TapiocaLpb. plantarum subsp. argentoratensis DK36
Fermented milletLpb. plantarum subsp. argentoratensis CNRZ1890
OgiLpb. plantarum subsp. argentoratensis NCIMB12120
Altamura breadLpb. plantarum PA20S, PE2S
Carasau breadLpb. plantarum subsp. plantarum 1069, 872
Cornetto di Matera breadLpb. paraplantarum MTG8L, MTG30L; Lpb. plantarum MT2A11S, MT2D3S; Lpb. plantarum subsp. argentoratensis MTC13L; Lpb. plantarum subsp. plantarum: MTD12L, MT2D20S, MTNTA3S, MT2D6S, MT2D7S, MT2D25L, MT2S, MTF13S, MTF1L, MTF28L, MTF9L
Moddizzosu breadLpb. plantarum subsp. plantarum 954
Spianata breadLpb. plantarum subsp. plantarum 1089
Zichi breadLpb. plantarum subsp. plantarum 1505, 1513
Wine (W)WineLpb. plantarum B161
Lpb. plantarum subsp. plantarum UT2.1, US3.1, UBS3
Human (H)HumanLpb. plantarum WCFS1
SalivaLpb. plantarum subsp. plantarum NCIMB8826
Unknown (U)UnknownLpb. plantarum subsp. plantarum S2A19LPa
* Strains isolated and identified in this study. # Strains from the Microbial Culture Collection of the Department of Food Science, University of Naples Federico II, Portici, Italy. The other strains belong to the Microbial Culture Collection of Industrial Microbiology Laboratory, University of Basilicata, Potenza, Italy.
Table
Table 2. Strain survival after exposure (15 min) to different concentrations of olive mill wastewater (OMW) derived from olive oil production of Leccino, Coratina and Cima di Melfi cultivars.
Table 2. Strain survival after exposure (15 min) to different concentrations of olive mill wastewater (OMW) derived from olive oil production of Leccino, Coratina and Cima di Melfi cultivars.
StrainsSpeciesDose Causing ≥ 7 log Reductions a
OMW b Leccino OMW b CoratinaOMW b
Cima di Melfi
O17Lpb. pentosus502550
O18Lpb. pentosus2512.550
OM24Lpb. pentosus12.512.550
OM53Lpb. pentosus256.2550
OM52Lpb. pentosus6.256.2525
OM62Lpb. pentosus6.256.2525
OM50Lpb. pentosus6.256.2525
OM13Lpb. pentosus12.56.2525
OM14Lpb. pentosus6.2512.525
2TPLpb. pentosus12.56.2525
MT2A11SLpb. plantarum252525
WCFS1Lpb. plantarum12.56.2525
C17Lpb. plantarum subsp. plantarum12.52525
ISLCPT57Lpb. plantarum subsp. plantarum6.253.1212.5
MTC13LLpb. plantarum subsp. argentoratensis12.56.2512.5
a The concentration of cells used to inoculate the different percentage (%) of OMW was 7 log cfu/mL. b OMW was diluted with NaCl 0.85% (w/v); the % of OMW corresponds to the following dilution (d): OMW 50% = 2d; OMW 25% = 4d; OMW 12.5% = 8d; OMW 6.25% = 16d; OMW 3.12% = 32d.
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Zotta, T.; Giavalisco, M.; Parente, E.; Picariello, G.; Siano, F.; Ricciardi, A. Selection of Lactiplantibacillus Strains for the Production of Fermented Table Olives. Microorganisms 2022, 10, 625. https://doi.org/10.3390/microorganisms10030625

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Zotta T, Giavalisco M, Parente E, Picariello G, Siano F, Ricciardi A. Selection of Lactiplantibacillus Strains for the Production of Fermented Table Olives. Microorganisms. 2022; 10(3):625. https://doi.org/10.3390/microorganisms10030625

Chicago/Turabian Style

Zotta, Teresa, Marilisa Giavalisco, Eugenio Parente, Gianluca Picariello, Francesco Siano, and Annamaria Ricciardi. 2022. "Selection of Lactiplantibacillus Strains for the Production of Fermented Table Olives" Microorganisms 10, no. 3: 625. https://doi.org/10.3390/microorganisms10030625

APA Style

Zotta, T., Giavalisco, M., Parente, E., Picariello, G., Siano, F., & Ricciardi, A. (2022). Selection of Lactiplantibacillus Strains for the Production of Fermented Table Olives. Microorganisms, 10(3), 625. https://doi.org/10.3390/microorganisms10030625

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