ORIGINAL RESEARCH article
Sec. Food Microbiology
Volume 10 - 2019 | https://doi.org/10.3389/fmicb.2019.00174
Effect of Sequential Inoculum of Beta-Glucosidase Positive and Probiotic Strains on Brine Fermentation to Obtain Low Salt Sicilian Table Olives
- 1Department of Agricultural, Food and Environment, University of Catania, Catania, Italy
- 2Department of Life Sciences, University of Modena and Reggio Emilia, Reggio Emilia, Italy
- 3Council for Agricultural Research and Economics, Research Centre for Olive, Citrus and Tree Fruit, Acireale, Italy
- 4Department of Agricultural, Food and Forest Science, University of Palermo, Palermo, Italy
- 5Food Biotechnology Department, Instituto de la Grasa, Consejo Superior de Investigaciones Científicas, Universidad Pablo de Olavide, Seville, Spain
In the present study, the β-glucosidase positive strain Lactobacillus plantarum F3. 3 was used as starter during the fermentation of Sicilian table olives (Nocellara Etnea cultivar) at two different salt concentrations (5 and 8%), in order to accelerate the debittering process. The latter was monitored through the increase of hydroxytyrosol compound. In addition, the potential probiotic Lactobacillus paracasei N24 strain was added after 60 days of fermentation. Un-inoculated brine samples at 5 and 8% of salt were used as control. The fermentation was monitored till 120 days through physico-chemical and microbiological analyses. In addition, volatile organic compounds and sensorial analyses were performed during the process and at the end of the fermentation, respectively. Lactic acid bacteria and yeasts were, in depth, studied by molecular methods and the occurrence of the potential probiotic N24 strain in the final products was determined. Results highlighted that inoculated brines exhibited a higher acidification and debittering rate than control ones. In addition, inoculated brines at 5% of salt exhibited higher polyphenols (hydoxytyrosol, tyrosol, and verbascoside) content compared to samples at 8% of NaCl, suggesting a stronger oleuropeinolytic activity of the starter at low salt concentration. Lactobacilli and yeasts dominated during the fermentation process, with the highest occurrence of L. plantarum and Wickerhamomyces anomalus, respectively. Moreover, the potential probiotic L. paracasei N24 strain was able to survive in the final product. Hence, the sequential inoculum of beta-glucosidase positive and potential probiotic strains could be proposed as a suitable technology to produce low salt Sicilian table olives.
Among fermented vegetables, table olives are widespread in the Mediterranean area with increasing consumption in both European and non-European countries (International Olive Council, 2016). Olives are intrinsically health thanks to the high content of fiber, vitamins, and polyphenols which play a very important role, exhibiting pharmacological properties and antioxidants effects. In particular, hydroxytyrosol scavenges free radicals, inhibits human low-density lipoprotein (LDL) oxidation, inhibits platelet aggregation, and discloses anticancer activity by means of pro-apoptotic mechanisms (Raederstorff, 2009; Allouche et al., 2011; Buckland and Gonzalez, 2015).
In Sicily, table olives fermentation is mainly performed under traditional methods exploiting the fermentative action of the autochthonous microbiota. Olives are directly brined without previous debittering treatment; therefore, the indigenous microorganisms and the effect of the physico-chemical conditions of brine (pH, salt, presence/absence O2, etc.) are mainly responsible of the hydrolysis of the oleuropein and of other β-glucosides. The oleuropein, a β-glucoside compound lending the strong “bitterness” aroma to the olive fruit, is hydrolyzed by β-glucosidases enzymes with the release of glucose and aglycones which are degraded, by an esterase, in the no-bitter phenols hydroxytyrosol, and elenolic acid (Bianchi, 2003). The spontaneous debittering is time consuming and not predictable, and it is strongly influenced by physico-chemical parameters, by the presence of fermentable substrates, and by the autochthonous microbiota. Starter cultures with oleuropein degrading activity were extensively applied in order to reduce the debittering time and to control the fermentation process (Panagou et al., 2003, 2008; Marsilio et al., 2005; Servili et al., 2006; Bevilacqua et al., 2013; Bonatsou et al., 2015), and, among them, the use of β-glucosidase positive strains could be promising (Ghabbour et al., 2011; Tataridou and Kotzekidou, 2015).
Recently, salt intake consumption hypertension and cardiovasular diseases [U.S. Dept. of Agriculture and U.S. Dept. of Health and Human Services, 2010; World Health Organization (WHO), 2012].
Recently, high attention was paid to salt intake since its overmuch intake is considered a risk factor for the onset of hypertension and cardiovascular diseases [U.S. Dept. of Agriculture and U.S. Dept. of Health and Human Services, 2010; World Health Organization (WHO), 2012]. Indeed, the set-up of table olives with low NaCl content is an issue of great interest for the sector (Bautista-Gallego et al., 2013a). However, a complete removal of salt may lead to an increased risk in the survival/ growth of spoilage or food pathogen microorganisms and may also alter food flavor, causing important economic losses. Hence, several studies evaluated the use of KCl, CaCl2, and ZnCl2 as NaCl replacers. It is well-demonstrated that table olives dealt with NaCl reduction and partial substitution with other salts have a more equilibrated mineral composition, enhancing the consumers' acceptance (Bautista-Gallego et al., 2010, 2011a, 2013b). Nevertheless, the effect of NaCl replaces on sensorial aspects is still controversial and strongly influenced by the concentration of the salt mixture used (Zinno et al., 2017). Recently, Pino et al. (2018a) demonstrated that the reduction of NaCl content to 5%, without any NaCl replacers, did not negatively affect the Nocellara Etnea table olives fermentation, obtaining a microbiologically safe product with appreciate sensorial traits.
Another challenge for vegetable product industry is to satisfy the increasing consumer demand for healthier products. Numerous studies demonstrated that table olives are promising carrier for probiotic strains being able to support their survival, probably thanks to the release of prebiotic substances from fruits. Additionally, their microstructure, in terms of roughness of olive surface, promotes the formation of biofilm that seem to protect probiotic bacteria from stressful conditions (such as acidic environment), favoring their survival through the human gastrointestinal tract (De Bellis et al., 2010; Arroyo-López et al., 2012a; Blana et al., 2014; Randazzo et al., 2017; Rodríguez-Gómez et al., 2017). According to that, the present study was aimed to evaluate the effect of a sequential inoculum of a β-glucosidase positive strain and probiotic bacteria on brine fermentation in order to set up a low salt Sicilian table olives.
Materials and Methods
Pilot Scale Olives Processing
Traditionally Sicilian–style table olives from Nocellara Etnea cultivar, provided from a local company, located in Paternò (Sicily), were processed without any lye treatment. Olives were pre-treated as previously reported (Pino et al., 2018a) and directly immersed in sterilized brine, containing 5 or 8% (w/v) of NaCl. The β-glucosidase positive strain Lactobacillus plantarum F3.3, previously isolated from fermented table olives was used as starter. The strain was previously characterized for the presence of bglH gene according to Marasco et al. (1998) and its β-glucosidase activity was evaluated by enzymatic assay, according to Sestelo et al. (2004). To set-up probiotic table olives, the potential probiotic Lactobacillus paracasei N24, belonging to the Di3A microbial collection was added. This strain was selected according to its technological and probiotic features (Pitino et al., 2010; Randazzo et al., 2010) and for its good ability to survive in table olives (Randazzo et al., 2017; Pino et al., 2018a). Both microorganisms were applied as lyophilized strains.
The experimental fermentation design comprised 8 treatments: 4 fermentations at 5% of NaCl with (F5A; F5B) and without (F5C; F5D) the addition of L. plantarum F3.3 strain, and 4 fermentations at 8% of NaCl with (F8A; F8B) and without (F8C; F8D) the addition of L. plantarum F3.3. Brine samples F5A; F5B; F8A; F8B were inoculated with the L. plantarum starter culture, to a final cell density of 7 log cfu/ml, directly after brining. The potential probiotic L. paracasei N24 strain was inoculated in F5B; F5D; F8B; F8D samples after 60 days of brining (at final cell density of 9 log cfu/ml). All fermentations were done at room temperature (18 ± 2°C), and followed up to 120 days. Marine salt was periodically added to maintain the initial concentration and fresh brine was supplied to keep olives totally dipped. Each fermentation was carried out in triplicate.
The pH of the brines was detected by using a MettlerDL25 pHmeter (MettlerDL25, Mettler-Toledo International Inc.). Titratable acidity was determined by titring brine samples with 0.1 N NaOH and was expressed as lactic acid (g/100 ml).
The olive brines were filtered through PTFE filters (Millipore, 0.45 μm) and injected in the chromatographic system to analyze the phenol fraction. The HPLC instrument consisted of a chromatography Waters Alliance 2695 HPLC equipped with a Waters 996 photodiode array detector (PDA) set at 280 nm. The column used was a Luna C18 (250 mm × 4.6 mm i.d., 5 μm, 100 Å, Phenomenex, Torrence, CA) which was maintained at 30°C in an oven. The flow rate was 1 mL/min. Separation was obtained by elution gradient using an initial composition of 95% of A solution (2% acetic acid in water) and 5% of B solution (methanol). The concentration of B solution was increased to 30% in 15 min and to 70% in 25 min and then, after 2 min in isocratic condition, the mobile phase was set at the same initial concentration in 8 min. Phenolic compounds were identified by injecting the pure standards of oleuropein, verbascoside, tyrosol, and hydroxytyrosol and by comparing their retention time and UV-Vis spectra. All the analyses were performed in triplicate.
Brine samples at 1, 30, 60, 90, and 120 days of fermentation were subjected to microbiological analysis as previously described (Pino et al., 2018a). Mannitol Salt Agar (MSA), incubated at 32°C for 48 h, was used to isolate both coagulase positive and negative staphylococci. All media were provided from Oxoid (Italy) with the exception of YM provided from Difco (Italy). Microbiological analyses were performed in triplicate and results were expressed as log cfu/ml ± standard deviation.
LAB Isolation and Identification
For each brine sample (F5A, F5B, F5C, F5D, F8A, F8B, F8C, and F8D) and each sampling time (1, 30, 60, 90, and 120 days), 20% of the total number of colonies, recovered on MRS agar plate, were randomly selected, purified, checked for catalase activity and Gram reaction, and microscopically examined before storing in liquid culture using 20% (v/v) glycerol at −80°C. Six-hundred (600) LAB isolates were purified and subjected to total genomic DNA (gDNA) extraction following the method described by Pino et al. (2018b). gDNA concentration and quality were evaluated using the Fluorometer Qubit (Invitrogen, Carlsbad, 278 CA, USA). Multiplex RecA and Tuf gene species-specific PCR were performed as previously described (Torriani et al., 2001; Ventura et al., 2003), respectively. Strains not identified at species level with species-specific PCR were subjected to 16S rRNA gene PCR-RFLP analysis according to Pino et al. (2018b). For each PCR-RFLP cluster, the 16S rRNA gene PCR amplicon of one representative strain was purified using the Qiaquick PCR purification kit (Qiagen Hilden, Germany) and was subjected to sequencing and Blast analysis.
Isolation and Genotypic Identification of Yeasts
From each brine samples at each sampling time, as previously reported, 200 colonies were randomly isolated from YM medium, purified, and microscopically examined prior to storing in liquid culture using 20% (v/v) glycerol at −80°C. For the yeasts characterization, DNA was extracted according to Ruiz-Barba et al. (2005) and subjected to repetitive element palindromic (rep)-PCR analysis by using GTG5 primer. The PCR reaction was carried out in a final volume of 25 μl, containing: 5 μl of DNA, 5 μl 5X PCR Buffer, 1 μl of primer GTG5 (5-GTGGTGGTGGTGGTG-3), 13.9 μl of filtered water on 0.1 μl of Taq polymerase (Invitrogen, Italy). The amplification program was as follows; an initial denaturation (95°C, 5 min) followed by 30 cycles of denaturation (95°C, 30 s), annealing (40°C, 1 min), and extension (65°C, 8 min) with a single final extension (65°C, 16 min). PCR products were electrophoresed in a 2 % agarose gel in 1X TAE buffer, stained with ethidium bromide (30 min) and visualized under ultraviolet light. The resulting fingerprints were digitally captured and analyzed with the Bionumerics 6.6 software package (Applied Maths, Kortrijk, Belgium). Dendrogram for clustering comparison was built with UPGMA (Unweighted Pair Group Method) method and Pearson correlation.
To validate the clustering analysis and for identification of strains, the 26S rDNA gene of all isolates was further sequenced. The gDNA amplification was performed according to Porrua et al. (2018). PCR products were resolved by electrophoresis on agarose gel (1% w/v) stained with ethidium bromide. DNA ladder plus (Invitrogen, USA) was used to evaluate the molecular weight of amplified DNA. PCR products were purified using Isolate DNA kit (Bioline, USA) according to the manufacturer's instructions and quantified by agarose gel electrophoresis (1% w/v) in 0.5X TBE buffer (89 mM Tris-borate, 2 mM EDTA pH 8). An amount of 10 μl of purified product with forward primer NL1 was used for sequencing by Stab Vida (Lisbon, Portugal). Nucleotide sequences were aligned with the software Molecular Evolution Genetic Analysis (MEGA).
Rep-PCR for Detecting the Presence of Probiotic L. paracasei N24 Strain
Rep-PCR genomic fingerprinting was performed on 79 L. paracasei strains, isolated from F5B, F5D, F8B, and F8D brine samples at 120 days of fermentation, using the (GTG)5-primer, as described by Versalovic et al. (1994). PCR was carried out in a 20 μl reaction mixture containing 1x Thermo Green buffer (Thermo Scientific, Waltman, MA, USA), 3.0 mM MgCl2, 200 μM of each dNTP (Fermentas), 1 U of Taq polymerase (Thermo Scientific, Waltman, MA, USA), 2 μM (GTG)5 primer and 50 ng gDNA. Amplifications were performed in a MyCycler thermal cycler (BioRad, Hercules, CA). The PCR cycling parameters and gel running conditions were set according to Solieri et al. (2012). The only modification was the change of annealing temperature from 40 to 45°C. The GeneRuler 100 bp Plus DNA Ladder (Thermo Scientific, Waltman, MA, USA) was used as a molecular size marker. BioDoc Gel Analyzer device (Biometra GmbH, Germany) was used to capture DNA fingerprint images which were then processed through the BioNumerics software v3.0 (Applied Maths, Sint-Martens-Latem, Belgium). Repeatability of rep-PCR was assessed using the inoculated strain N24 as internal control. Pearson's correlation similarity coefficient was chosen to calculate bands patterns similarity matrix with optimization and curve smoothening values at 1%. Unweighted pair group method with arithmetic mean (UPGMA) analysis was exploited to build the (GTG)5-based dendrogram.
Analysis of Volatile Organic Compounds (VOCs)
VOCs analysis was performed on brine samples at 1, 60, and 120 days of fermentation following method and conditions previously described (Randazzo et al., 2017; Pino et al., 2018a) using a gas chromatography-mass-spectrometry (GC-MS). All analyses were performed in triplicate and the results were expressed as means in μg/l of brine.
Sensory Evaluation of Table Olives
Table olives at 120 days of fermentation were subjected to sensory evaluation by trained panelists (6 females and 4 males, aged from 22 to 40 years). Sensory panel was conducted according to the International Olive Council method (International Olive Council, 2011). Descriptors related to negative sensations, gustatory, and kinaesthetic perceptions were evaluated as previously described (International Olive Council, 2011, 2016; Pino et al., 2018a). In addition, the overall acceptability descriptor, such an indication of the overall quality, was also scored. Sensory data were acquired by a direct computerized registration system (FIZZ Biosystemes. Couternon, France).
Microbiological and chemical (i.e., single phenol compounds, pH and acidity) data were analyzed by ANOVA (One-way Analysis of Variance) using Tukey's post-hoc test, in order to assess the overall differences among treatments. The reference level of significance was 0.01 for chemical assay and 0.05 for VOCs and microbiolgical assays. All statistical analyses were performed using MATLAB software (MathWorks, version 8.5.0), while sensory data were analyzed using the software package Statgraphics® Centurion XVI (Statpoint Technologies, INC.) setting samples as treatments. Data correlations between brine samples differently treated and VOCs were computed using XLStat software (version 2016.1).
In Table 1, the results of pH and titratable acidity detected in brine samples analyzed thought the fermentation are shown. At the beginning of fermentation, pH values ranged from 5.8 to 6.3, and then they decreased after 30 days. Differences among samples become more appreciable after 60 days of fermentation with the lowest values showed by F5B and F8C samples. At the end of fermentation (120 days) the pH fitted the hygienic limit of 4.3 in all samples (Table 1).
Table 1. Results of pH and titratable acidity values in olive brines expressed as means and standard deviations at different time of fermentations.
The titratable acidity values exhibited an increasing trend in all samples with the exception of F8A and F8B brines, which slightly decreased in acidity at 120 days. The highest acidity values were detected in brines at 5% of NaCl (F5A, F5B, F5C, and F5D). In addition, a significant increase in acidity was recorded after the addition of N24 strain (90 days) mainly in F5B and F5D samples (Table 1).
Results of hydroxytyrosol, tyrosol, oleuropein, and verbascoside quantification are shown in Table 2. Overall, all polyphenols analyzed showed an increasing trend during the fermentation mainly in 5% NaCl brine samples inoculated with starter culture. The highest values of hydroxytyrosol, tyrosol, and verbascoside were mainly recorded in brines inoculated with L. plantarum F3.3 starter culture already at 30 days. Similar behavior was observed for oleuropein.
Table 2. Results of the analyzed phenols in olive brines expressed as means (mg/l) and standard deviations at different time of fermentations.
Table 3 shown microbial counts of brine samples at both 5 and 8% of NaCl, which is expressed as log cfu/ml. Viable mesophilic bacteria showed different trend among samples. In detail, brines at 5% of NaCl (F5A–F5D), from an initial average value of 7.11 log unit, exhibited a steady trend during the fermentation with slight decrease of cell density after 60 days. Similar behavior was observed for brine samples at 8% of NaCl (F8A–F8D) which showed a mean initial value of 6.73 log unit and a final mean value of 5.56 log unit (Table 3). Regarding LAB population, all brine samples inoculated with starter culture (F5A, F5B, F8A, F8B) presented, at the beginning of fermentation, higher cell density than spontaneous ones (F5C, F5D, F8C, F8D). From 60 to 120 days, LAB reached the highest values in samples inoculated with the potential probiotic N24 strain (F5B, F5D, F8B, F8D). Yeasts were present at an initial level of about 3 log cfu/ml in all experimental brines with the exception of F5A and F5B samples which exhibited initial value of 4.04 and 4.37 log cfu/ml, respectively (Table 3). The yeasts cell densities significantly increased thought the fermentation process, achieving, at 120 days, an average value of 7.37 log unit and 6.64 log unit in brine samples at 5 and 8% of NaCl, respectively. Regarding the staphylococci count, only coagulase negative staphylococci, forming red colonies in the medium, were enumerated and their level, at the beginning of the fermentation, was quite similar among all samples. After a slight increase till 60 days, a decrease to final average values of 3.0 and 3.8 log cfu/ml was achieved in 5 and 8% brine samples, respectively. Similar behavior was observed for enterobacteria counts, which significantly decreased through the fermentation process. At the end of fermentation (120 days) this microbial group was detected, at value below 2 log, in brine samples at 8% of NaCl and below the detection limit in samples at 5% of NaCl, with the exception of the F5D sample. E. coli was never detected in any brine samples analyzed (data not shown).
Table 3. Microbial counts expressed as log10 CFU/ml of 3 replicates ± standard deviation of the main microbial groups detected in experimental brine samples during the fermentation process.
Molecular Identification of LAB
Six hundred isolates from MRS agar plates were considered LAB based on their positive Gram reaction, non-motility, absence of catalase activity and spore formation, as well as rod or coccal shape. RecA and Tuf gene species-specific PCRs revealed the presence of strains belonging to L. plantarum, Lactobacillus pentosus, L. paracasei, and Lactobacillus casei species. The distribution of lactobacilli at different sampling times is reported in Figure 1A and their occurrence in the different brine samples is showed in Figure 1B. Isolates not identified at species level were indicated as “others.” Evaluating the distribution of LAB strains through the fermentation, results indicated that L. plantarum and L. pentosus represented the dominant species at the beginning of the process (till 30th days) and a high occurrence of L. paracasei species was detected up to 60 days. Whereas, the highest occurrence of L. casei strains was achieved at 120 days (Figure 1A). Zooming on the fermentation at different salt content (5 and 8%) differently inoculated, results showed the dominance of L. plantarum strains in samples inoculated with starter, the highest occurrence of L. casei and L. pentosus in spontaneous samples (F5C, F8C, F5D, F8D) and of L. paracasei in samples inoculated with the probiotic strain N24 (Figure 1B).
Figure 1. Isolation frequency, expressed in percentage, of LAB species throughout the fermentation (A) and in the experimental brine samples (B).
Isolates not identified initially with recA and Tuf gene primer pairs were subjected to PCR-RFLP analysis of the 16SrDNA and clustered into four different groups (data not shown). One representative isolate for each cluster was identified by 16S rRNA gene sequencing and were deposited in the GenBank database. The species attribution and the accession numbers of the sequenced strains were as follows (isolates code in parentheses): Leuconostoc mesenteroides MK085109 (F5C.1), Lactococcus lactis MK085110 (F5B.38), Lactobacillus brevis MK085111 (F5D.44), and Enterococcus faecium MK085112 (F5A.21).
Molecular Identification of Yeasts
Two-hundred yeast isolates were randomly obtained during the fermentation process. The dendogram generated by rep-PCR with primer GTG5 showed that the isolates formed 17 groups clearly differentiated. The most numerous groups belonged to the Wickerhamomyces anomalus and Candida boidinii species, although representatives of Candida diddensiae, Pichia kluyveri and Meyerozyma guillermondii were also identified (Figure 2A).
Figure 2. Dendrogram generated after bioinformatics analysis with Bionumerics 6.6 software package of the rep-PCR profiles obtained with GTG5 (A). Isolation frequency (%) of yeasts during the fermentation time of Nocellara Etnea table olives (B). Distribution of yeast species in different experimental brine samples (C).
The evolution of the different yeast species throughout the fermentative process is presented in Figure 2B. At this regard, W. anomalus and C. boidinii formed a stable dual species consortium through the fermentation, since they were both detected more frequently than others species, with a mean frequency of 49 and 37%, respectively. Indeed, these species were dominant in all brine samples differently treated (Figure 2C). The rest of the species were isolated at very low mean frequencies; in particular, M. guillermondii (1.97%) was detected only in samples at 8% of NaCl till 30th days of fermentation, whereas, P. kluyveri (2.98%) in samples F5A, F5D, and F8D till 60 days and C. diddensiae (5.87%) was detected starting from the 30th day of fermentation only in brines at 8% of NaCl (Figure 2C).
Detection of L. paracasei N24 Strain at 120 Days of Fermentation
The presence of inoculated strain N24 was assessed at 120 days of fermentation by rep-PCR with primer GTG5 on a pool of 79 L. paracasei isolates from samples F5B, F5D, F8B, and F8D. Preliminarily, the rep-PCR repeatability was evaluated using gDNA from strain N24 as internal control in four different gels, obtaining a similarity of 74.3% (data not shown). Accordingly, this value was retained as similarity threshold to establish the identity of isolates compared to the rep-PCR profile of promising probiotic strain N24. The dendrogram generated using the GTG5-based patterns of L. paracasei isolates revealed the presence of four major clusters (from A to D) and four singleton L. paracasei isolates below 74.3% similarity (Figure 3; Supplementary Figure 1). The cluster analysis showed that the major cluster A grouped both the inoculated strain N24 and 48 out of 79 isolates, indicating that these isolates were assimilated to the N24 strain profile. The majority of them were isolated from samples F5B and F8B, over the indigenous L. paracasei isolates. In detail, out of 48, 18 strains were isolated from F5B, 12 from F8B, 10 from F5D, and 8 from F8D. The remaining isolates belonged to clusters B, C, and D.
Figure 3. Dendrogram generated after cluster analysis of the digitized GTG5-PCR fingerprints of the Lactobacillus paracasei strains isolated from F5B, F5D, F8B, and F8D brine samples at 120 days of fermentation.
Volatile Organic Compounds (VOCs)
Results of VOCs of different brine samples at 60 and 120 days of fermentation are reported in Table 4. Overall, 46 compounds as acids, alcohols, esters, aldehydes, and phenols were identified, exhibiting a growing trend through the fermentation, with the exception of samples F5A, F5D, F8A, and F8D. The highest value was registered in samples F8C, with a value of 2,739.17 μg/l. Alcohols were the most abundant compounds, followed by esters and acids, whereas aldehydes and phenols were detected at lower concentrations. Focusing on each compound, among alcohols, ethanol dominated the fermentation process showing an increase only in spontaneous samples (F5C and F8C), followed by isoamylalcohol and phenylethylalcohol, which registered a variable trend through the fermentation (Table 4). Ethyl-acetate and methyl 2-methylbutanoate were the main detected esters. Among acids, the acetic acid was the most abundant compound, with the highest value in F5C and F8C samples. The most abundant aldehydes and phenols were nonanal, benzaldehyde and creasol, respectively (Table 4).
Table 4. Volatile organic compounds (VOCs) expressed as μg/l of experimental brine samples at 60 and 120 days of fermentation.
Figure 4 shows correlation between VOCs and brine samples differently treated. Overall, it is possible to point out that the salt concentration did not influence the VOCs formation through fermentation in brine samples, which were mainly grouped based on the treatment (starter and/or probiotic addition and spontaneous). In detail, samples inoculated with starter (F5A and F8A) were clustered together, showing a negative correlation with alcohol and ester compounds; spontaneous brine samples inoculated with the probiotic strain N24 (F5D and F8D) were negatively correlated to phenols, aldehydes and alcohols. Different correlations were detected for samples inoculated with both starter and probiotic strains (F5B and F8B). In particular, sample F8B at 60 and 120 days of fermentation were grouped together, exhibiting a positive correlation with alcohols and acids and a negative correlation with phenols and aldehydes (Figure 4). Evaluating sample F5B, it is possible to assert that VOCs formation was strongly influenced by the fermentation time. In fact, the sample F5B at 120 days revealed a distinct VOCs profile, displaying a positive correlation with esters, acids, and phenols. Similarly, spontaneous fermentation samples (F5C and F8C) were grouped based on fermentation time, showing a divergent VOCs profile through the fermentation.
Figure 4. Heat map of correlation between VOCs and F5 (A-D) and F8 (A-D) brine samples at 60 and 120 days of fermentation. The colors of the scale bar denote the nature of the correlation, with 1 indicating a perfectly positive correlation (green) and −1 indicating a perfectly negative correlation (red) between VOCs and brine samples.
Table 5 shown results of sensory analysis. Overall, none negative sensation was perceived, as deduced by the low scores attributed by panelist to these descriptors. No statistically significant differences were achieved among samples for hardness, fibrousness, and crunchiness. Among gustatory descriptors, higher scores for acidity were attributed to un-inoculated brine samples at both 5 and 8% of NaCl (F5C and F8C), while higher bitterness score was observed in samples without the addition of the β-glucosidase L. plantarum strain (F5C, F5D, F8C, and F8D). Finally, F5B and F8B samples received higher scores for the overall acceptability descriptor.
A current challenge in the processing technology of table olives is the selection of starter cultures able to fasten and safely drive the fermentation process. In contrast to industrial starter cultures, autochthonous strains, that naturally dominate spontaneous fermentation, tend to have high metabolic capacities, which can beneficially affect the quality of the final product. In addition, it was already established that the microbial dynamics through fermentation is influenced by the technology applied (e.g., salt reduction). One of the most widely employed strategies to reduce sodium content in table olives is the use of NaCl substitutes, which can be added alone or in combination with other salts (Bautista-Gallego et al., 2013a). Few studies have evaluated the possibility to setup low NaCl table olives without any salt replacement. Based on our previously reported data (Randazzo et al., 2017; Pino et al., 2018a), in the present study a wild β-glucosidase positive strain was used both as debittering and as driven agent during olive fermentations at lowered salt content (5%). It is well-known that β-glucosidase enzyme is important for oleuropein hydrolysis and, among lactobacilli, L. plantarum species has been successfully used as starter for its strong ability to break the glycosidic bond of oleuropein (Ciafardini et al., 1994; Tataridou and Kotzekidou, 2015) and for its high versatility. Overall, our data revealed that all brine samples reached a pH value ≤ 4.3 and exhibited a good acidification rate, indicating the success of the fermentation and ensuring the microbiological safety of the final product, in accordance to other researches (Corsetti et al., 2012; Martorana et al., 2017). In particular, samples inoculated with the β-glucosidase positive strain exhibited a more pronounced reduction of the fermentation time, with a higher content of hydroxytyrosol, tyrosol, and verbascoside compounds from 30 days of fermentation than un-inoculated ones, according to other studies (Romero et al., 2004; Ben Othman et al., 2009; Pistarino et al., 2013; Kaltsa et al., 2015). In addition, the autochthonous strain exhibited a better adaptation/growth rate in brine samples at 5% of salt. It is well-established that autochthonous strains are generally more adapted to harsh conditions of raw material than allochthonous ones, and, therefore, to dominate the microbiota, driving the fermentation and counteracting spoilage microorganisms (Di Cagno et al., 2008; Bevilacqua et al., 2015). Microbiological data indicated a significant reduction of Enterobacteriaceae starting from 30 days of fermentation, with an improvement of the safety of the final product, as previously reported (Pino et al., 2018a). It is interesting to point out that results revealed a high occurrence of yeasts as part of table olive natural microbiota, coexisting with LAB during the whole fermentation process (Arroyo-López et al., 2008, 2012a,c), which could be related to the geographic area, and cultivars (Bleve et al., 2014). Our data registered an unusual yeast count at the end of the process, higher than Spanish-style and Sicilian-style table olives, which generally reached value of 4-5- log CFU/ml. This could be linked to the processing technology applied in the present study. Yeasts favor bacteria growth, enhancing lactic acid production to inhibit spoilage microorganisms and affect flavor and texture of the final products (Arroyo-López et al., 2008, 2012b; Bevilacqua et al., 2013). As reported in a recent review, Candida boidinii, Debaryomyces hansenii, and Pichia membranifaciens were revealed as the most geographically diffused species (Campus et al., 2018). Evaluating yeast behavior, although it is noteworthy that yeast development is related to high salt level and phenolic compounds or low pH. In the present study, W. anomalus, and C. boidinii were the species mainly detected in brines processed at 5% of salt, whereas C. diddensae and M. guilliermondii were mainly revealed in brines at 8% NaCl. Several studies reported strong β-glucosidase activity for W. anomalus species (Bautista-Gallego et al., 2011b; Arroyo-López et al., 2012c; Romero-Gil et al., 2013; Bonatsou et al., 2015), and strong lipase and esterase activities for C. boidinii species, which positive impacts to fruity and olive flavor (Hernández et al., 2007; Bautista-Gallego et al., 2011b; Arroyo-López et al., 2012c; Pereira et al., 2015). In contrast to previously published data (Hurtado et al., 2008; Bautista-Gallego et al., 2011b), C. diddensae, which is generally associated to the early stage of fermentation, was detected at the highest frequency at 120 days. Focusing on LAB population, L. plantarum, L. pentosus, and L. paracasei were the main species found in all brine samples, confirming both their key role in table olive fermentation and biofilm formation with yeasts. In addition, a high survivability of the potential probiotic L. paracasei N24 strain was depicted in the final products, mainly in samples at 5% of NaCl. This evidence confirms its suitability to growth in harsh environment, such as brines, and that table olives are able to support probiotic survival (Lavermicocca et al., 2005; Rodríguez-Gómez et al., 2017; Pino et al., 2018a). In fact, nutrients and prebiotics released into the brines favor the biofilm formation, protecting bacteria from acidic environment and enhancing their passage through human gastrointestinal (GI) tract (De Bellis et al., 2010; Ranadheera et al., 2010; Arroyo-López et al., 2012a; Blana et al., 2014; Rodríguez-Gómez et al., 2014a,b, 2017; Grounta et al., 2015). It is interesting to point out that the addition of the potential probiotic strain at 60 days of fermentation in brine samples processed at low salt content and with starter, significantly modified the VOCs pattern. In particular, compounds responsible for floral and fruity notes, such as phenylethyl alcohol and methyl 2-methylbutanoate, highly increased, while ethanol and isoamyl-alcohol significantly deceased compared to un-inoculated samples. The high content of alcohols in un-inoculated brine samples could be related to yeast metabolic activities (Bleve et al., 2014; Randazzo et al., 2017). This evidence was in accordance to sensory data since panelists attributed the higher score to the bitterness and acid descriptors in un-inoculated samples. Finally, data obtained from correlation between VOCs and brine samples differently treated revealed that the VOCs formation was mainly influenced by the starter and/or probiotic addition instead of salt content.
The effects of a sequential inoculum of β-glucosidase positive and potential probiotic strains on the fermentation of Sicilian table olives were investigated. Remarkably, results demonstrate that the technology applied, based on the sequential inoculum and the brines fermentation at low salt content, without any salt replacement, did not increase the risk of microbial spoilage, nor the overgrowth of foodborne pathogens. Indeed, the composition and the dynamics of brine microbiota, mainly constituted by LAB and yeasts consortium, significantly affected the composition of the VOCs and the sensorial traits of the final products, which were confirmed by a panel of trained assessors. Hence, the results of the present study are promising, suggesting the possibility to formulate table olives with reduced salt content.
AP, FR, AT, AV, and LS performed the experiments and analyzed the data. AP, JB-G, and CR wrote the manuscript. CR, JB-G, and CC designed the study. CR, JB-G, and FA-L contributed to data interpretation. All authors revised the manuscript.
Conflict of Interest Statement
The authors declare that the research was conducted in the absence of any commercial or financial relationships that could be construed as a potential conflict of interest.
We thanks Dr. Vincenzo Alfeo for his advice on VOCs determination and statistical analysis. LS was supported by the Italian Ministry of Education, University, and Research (MIUR), within the framework of the Italian National Grant for Fundamental Research (FFABR 2017). JB-G thanks MINECO and CSIC for his JDC-Incorp. fellowship. The research was supported by the Project Valutazione della sostenibilità dei sistemi agroalimentari locali e selezione di markers molecolari e biologici nella gestione della qualità di prodotti agroalimentari funded by the University of Catania (Italy).
The Supplementary Material for this article can be found online at: https://www.frontiersin.org/articles/10.3389/fmicb.2019.00174/full#supplementary-material
Allouche, Y., Warleta, F., Campos, M., Sanchez-Quesada, C., Uceda, M., Beltran, G., et al. (2011). Antioxidant, antiproliferative, and pro-apoptotic capacities of pentacyclic triterpenes found in the skin of olives on MCF-7 human breast cancer cells and their effects on DNA damage. J. Agric. Food Chem. 59, 121–130. doi: 10.1021/jf102319y
Arroyo-López, F. N., Bautista-Gallego, J., Domínguez-Manzano, J., Romero-Gil, V., Rodriguez-Gómez, F., García-García, P., et al. (2012a). Formation of lactic acid bacteria-yeasts communities on the olive surface during Spanish-style Manzanilla fermentations. Food Microbiol. 32, 295–301. doi: 10.1016/j.fm.2012.07.003
Arroyo-López, F. N., Bautista-Gallego, J., Duran-Quintana, M. C., Rodríguez-Gómez, F., Romero-Barranco, C., and Garrido-Fernández, A. (2008). Improvement of the storage process for cracked table olives. J. Food Eng. 89, 479–487. doi: 10.1016/j.jfoodeng.2008.06.001
Arroyo-López, F. N., Romero-Gil, V., Bautista-Gallego, J., Rodríguez-Gómez, F., Jiménez-Díaz, R., García-García, P., et al. (2012b). Potential benefits of the application of yeast starters in table olive processing. Front. Microbiol. 3:161. doi: 10.3389/fmicb.2012.00161
Arroyo-López, F. N., Romero-Gil, V., Bautista-Gallego, J., Rodríguez-Gomez, F., Jiménez-Díaz, R., García-García, P., et al. (2012c). Yeasts in table olive processing: desirable or spoilage microorganisms? Int. J. Food Microbiol. 160, 42–49. doi: 10.1016/j.ijfoodmicro.2012.08.003
Bautista-Gallego, J., Arroyo-Lopez, F. N., Duran-Quintana, M. C., and Garrido-Fernandez, A. (2010). Fermentation profiles of Manzanilla-Alorena cracked green table olives in different chloride salt mixtures. Food Microbiol. 27, 403–412. doi: 10.1016/j.fm.2009.11.015
Bautista-Gallego, J., Arroyo-López, F. N., Romero-Gil, V., Rodríguez-Gómez, F., Garcia-Garcia, P., and Garrido-Fernández, A. (2011a). Chloride salt mixtures affect Gordal cv. green Spanish-style table olive fermentation. Food Microbiol. 28, 1316–1325. doi: 10.1016/j.fm.2011.06.002
Bautista-Gallego, J., Moreno-Baquero, J. M., Garrido-Fernandez, A., and Lopez-Lopez, A. (2013b). Development of a novel Zn fortified table olive product. LWT-Food Sci. Technol. 50, 264–271. doi: 10.1016/j.lwt.2012.05.017
Bautista-Gallego, J., Rantsiou, K., Garrido-Fernández, A., Cocolin, L., and Arroyo-López, F. N. (2013a). Salt reduction in vegetable fermentation: reality or desire? J. Food. Sci. 78, 1095–1100. doi: 10.1111/1750-3841.12170
Bautista-Gallego, J., Rodriguez-Gomez, F., Barrio, E., Querol, A., Garrido-Fernandez, A., and Arroyo-López, F. N. (2011b). Exploring the yeast biodiversity of green table olive industrial fermentations for technological applications. Int. J. Food Microbiol. 147, 89–96. doi: 10.1016/j.ijfoodmicro.2011.03.013
Ben Othman, N., Roblain, D., Chammem, N., Thonart, P., and Hamdi, M. (2009). Antioxidant phenolic compounds loss during the fermentation of Chétoui olives. Food Chem. 116, 662–669. doi: 10.1016/j.foodchem.2009.02.084
Bevilacqua, A., De Stefano, F., Augello, S., Pignatiello, S., Sinigaglia, M., and Corbo, M. R. (2015). Biotechnological innovations for table olives. Int. J. Food Sci. Nutr. 66, 127–131. doi: 10.3109/09637486.2014.959901
Blana, V. A., Grounta, A., Tassou, C. C., Nychas, G. J. E., and Panagou, E. Z. (2014). Inoculated fermentation of green olives with potential probiotic Lactobacillus pentosus and Lactobacillus plantarum starter cultures isolated from industrially fermented olives. Food Microbiol. 38, 208–218. doi: 10.1016/j.fm.2013.09.007
Bleve, G., Tufariello, M., Durante, M., Perbellini, E., Ramires, F. A., Grieco, F., et al. (2014). Physico-chemical and microbiological characterization of spontaneous fermentation of Cellina di Nardò and Leccino table olives. Front. Microbiol. 5:570. doi: 10.3389/fmicb.2014.00570
Bonatsou, S., Benitez, A., Rodriguez-Gómez, F., Panagou, E. Z., and Arroyo-Lopez, F. N. (2015). Selection of yeasts with multifunctional features for application as starters in natural black table olive processing. Food Microbiol. 46, 66–73. doi: 10.1016/j.fm.2014.07.011
Buckland, G., and Gonzalez, C. A. (2015). The role of olive oil in disease prevention: a focus on the recent epidemiological evidence from cohort studies and dietary intervention trials. Br. J. Nutr. 113, S94–S101. doi: 10.1017/S0007114514003936
Corsetti, A., Perpetuini, G., Schirone, M., Tofalo, R., and Suzzi, G. (2012). Application of starter cultures to table olive fermentation: an overview on the experimental studies. Front. Microbiol. 3:248. doi: 10.3389/fmicb.2012.00248
De Bellis, P., Valerio, F., Sisto, A., Lonigro, S. L., and Lavermicocca, P. (2010). Probiotic table olives: microbial populations adhering on olive surface in fermentation sets inoculated with the probiotic strain Lactobacillus paracasei IMPC2.1 in an industrial plant. Int. J. Food Microbiol. 140, 6–13. doi: 10.1016/j.ijfoodmicro.2010.02.024
Di Cagno, R., Surico, R. F., Siragusa, S., De Angelis, M., Paradiso, A., Minervini, F., et al. (2008). Selection and use of autochthonous mixed starter for lactic acid fermentation of carrots, French beans or marrows. Int. J. Food Microbiol. 127, 220–228. doi: 10.1016/j.ijfoodmicro.2008.07.010
Ghabbour, N., Lamzira, Z., Thonart, P., Cidalia, P., Markaoui, M., and Asehraou, A. (2011). Selection of oleuropein-degrading lactic acid bacteria strains isolated from fermenting moroccan green olives. Grasas Aceites 62, 84–89. doi: 10.3989/gya.055510
Grounta, A., Doulgeraki, A. I., and Panagou, E. Z. (2015). Quantification and characterization of microbial biofilm community attached on the surface of fermentation vessels used in green table olive processing. Int. J. Food Microbiol. 203, 41–48. doi: 10.1016/j.ijfoodmicro.2015.03.001
Hernández, A., Martin, A., Aranda, E., Pérez-Nevado, F., and Córdoba, M. G. (2007). Identification and characterization of yeast isolated from the elaboration of seasoned green table olives. Food Microbiol. 24, 346–351. doi: 10.1016/j.fm.2006.07.022
Hurtado, A., Reguant, C., Esteve-Zarzoso, B., Bordons, A., and Rozès, N. (2008). Microbial population dynamics during the processing of Arbequina table olives. Food Res. Int. 41, 738–744. doi: 10.1016/j.foodres.2008.05.007
Kaltsa, A., Papaliaga, D., Papaioannou, E., and Kotzekidou, P. (2015). Characteristics of oleuropeinolytic strains of Lactobacillus plantarum group and influence on phenolic compounds in table olives elaborated under reduced salt conditions. Food Microbiol. 48, 58–62. doi: 10.1016/j.fm.2014.10.016
Lavermicocca, P., Valerio, F., Lonigro, S. L., De Angelis, M., Morelli, L., Callegari, M. L., et al. (2005). Adhesion and survival of lactobacilli and bifidobacteria on table olives with the aim of formulating a new probiotic food. Appl. Environ. Microbiol. 71, 4233–4240. doi: 10.1128/AEM.71.8.4233-4240.2005
Marasco, R., Muscariello, L., Varcamonti, M., De Felice, M., and Sacco, M. (1998). Expression of the bglH gene of Lactobacillus plantarum is controlled by carbon catabolite repression. J. Bacteriol. 13, 3400–3404.
Marsilio, V., Seghetti, L., Iannucci, E., Russi, F., Lanza, B., and Felicioni, M. (2005). Use of a lactic acid bacteria starter culture during green olive processing (Olea europaea L. cv. Ascolana tenera). J. Food Sci. Agric. 87, 1084–1090. doi: 10.1002/jsfa.2066
Martorana, A., Alfonzo, A., Gaglio, R., Settanni, L., Corona, O., La Croce, F., et al. (2017). Evaluation of different conditions to enhance the performances of Lactobacillus pentosusOM13 during industrial production of Spanish-style table olives. Food Microb. 61, 150–158. doi: 10.1016/j.fm.2016.08.007
Panagou, E. Z., Schillinger, U., Franz, C. M. A. P., and Nychasa, G. J. E. (2008). Microbiological and biochemical profile of cv. Conservolea naturally black olives during controlled fermentation with selected strains of lactic acid bacteria. Food Microbiol. 25, 348–358. doi: 10.1016/j.fm.2007.10.005
Panagou, E. Z., Tassou, C. C., and Katsaboxakis, C. Z. (2003). Induced lactic acid fermentation of untreated green olives of the Conservolea cultivar by Lactobacillus pentosus. J. Sci. Food Agric. 83, 667–674. doi: 10.1002/jsfa.1336
Pereira, E. L., Ramalhosa, E., Borges, A., Pereira, J. A., and Baptista, P. (2015). Yeast dynamics during the natural fermentation process of table olives (Negrinha de Freixo cv.). Food Microbiol. 46, 582–586. doi: 10.1016/j.fm.2014.10.003
Pino, A., De Angelis, M., Todaro, A., Van Hoorde, K., Randazzo, C. L., and Caggia, C. (2018a). Fermentation of Nocellara Etnea table olives by functional starter cultures at different low salt concentrations. Front. Microbiol. 9:1125. doi: 10.3389/fmicb.2018.01125
Pino, A., Liotta, L., Randazzo, C. L., Todaro, A., Mazzaglia, A., De Nardo, F., et al. (2018b). Polyphasic approach to study physico-chemical, microbiological and sensorial characteristics of artisanal Nicastrese goat's cheese. Food Microbiol. 70, 143–154. doi: 10.1016/j.fm.2017.09.005
Pistarino, E., Aliakbarian, B., Casazza, A. A., Paini, M., Cosulich, M. E., and Perego, P. (2013). Combined effect of starter culture and temperature on phenolic compounds during fermentation of Taggiasca black olives. Food Chem. 138, 2043–2049. doi: 10.1016/j.foodchem.2012.11.021
Pitino, I., Randazzo, C. L., Mandalari, G., Lo Curto, A., Faulks, R. M., Le Marc, Y., et al. (2010). Survival of Lactobacillus rhamnosus strains in the upper gastrointestinal tract. Food Microb. 27, 1121–1127. doi: 10.1016/j.fm.2010.07.019
Porrua, C., Rodríguez-Gómez, F., Benítez-Cabello, A., Jiménez-Díaz, R., Zara, G., Budroni, M., et al. (2018). Genotyping, identification and multifunctional features of yeasts associated to Bosana naturally black table olive fermentations. Food Microb. 69, 33–42. doi: 10.1016/j.fm.2017.07.010
Randazzo, C. L., Pitino, I., Ribbera, A., and Caggia, C. (2010). Bacterial population of Pecorino Crotonese cheese and its influence in flavour formation. Food Microbiol. 27, 363–374. doi: 10.1016/j.fm.2009.11.010
Randazzo, C. L., Todaro, A., Pino, A., Corona, O., and Caggia, C. (2017). Microbiota and metabolome during controlled and spontaneous fermentation of Nocellara Etnea table olives. Food Microbiol. 65, 136–148. doi: 10.1016/j.fm.2017.01.022
Rodríguez-Gómez, F., Romero-Gil, V., Arroyo-López, F. N., Roldán-Reyes, J. C., Torres-Gallardo, R., Bautista-Gallego, J., et al. (2017). Assessing the challenges in the application of potential probiotic lactic acid bacteria in the large-scale fermentation of Spanish-style table olives. Front. Microbiol. 8:915. doi: 10.3389/fmicb.2017.00915
Rodríguez-Gómez, F., Romero-Gil, V., Bautista-Gallego, J., García-García, P., Garrido-Fernández, A., and Arroyo-López, F. N. (2014a). Production of potential probiotic Spanish-style green table olives at pilot plant scale using multifunctional starters. Food Microbiol. 44, 278–287. doi: 10.1016/j.fm.2014.03.023
Rodríguez-Gómez, F., Romero-Gil, V., García-García, P., Garrido-Fernández, A., and Arroyo-López, F. N. (2014b). Fortification of table olive packing with the potential probiotic bacteria Lactobacillus pentosus TOMC-LAB2. Front. Microbiol. 5:467. doi: 10.3389/fmicb.2014.00467
Romero, C., Brenes, M., Yousfi, K., Garcia, P., Garcia, A., and Garrido, A. (2004). Effect of cultivar and processing method on the contents of polyphenols in table olives. J. Agric. Food Chem. 52, 479–484. doi: 10.1021/jf030525l
Romero-Gil, V., Bautista-Gallego, J., Rodríguez-Gómez, F., García-García, P., Jiménez-Díaz, R., Garrido-Fernández, A., et al. (2013). Evaluating the individual effects of temperature and salt on table olive related microorganisms. Food Microbiol. 33, 178–184. doi: 10.1016/j.fm.2012.09.015
Ruiz-Barba, J. L., Maldonado, A., and Jiménez-Díaz, R. (2005). Small-scale total DNA extraction from bacteria and yeast for PCR applications. Anal. Biochem. 347, 333–335. doi: 10.1016/j.ab.2005.09.028
Servili, M., Settanni, L., Veneziani, G., Esposto, S., Massitti, O., Taticchi, A., et al. (2006). 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. 54, 3869–3875. doi: 10.1021/jf053206y
Sestelo, A. B. F., Poza, M., and Villa, T. G. β-,Glucosidase activity in a Lactobacillus plantarum wine strain. (2004). World J. Microbiol. Biotechnol. 20, 633–637. doi: 10.1023/B:WIBI.0000043195.80695.17
Solieri, L., Bianchi, A., and Giudici, P. (2012). Inventory of non starter lactic acid bacteria from ripened Parmigiano Reggiano cheese as assessed by a culture dependent multiphasic approach. Syst. Appl. Microbiol. 35, 270–277. doi: 10.1016/j.syapm.2012.04.002
Tataridou, M., and Kotzekidou, P. (2015). Fermentation of table olives by oleuropeinolytic starter culture in reduced salt brines and inactivation of Escherichia coli O157:H7 and Listeria monocytogenes. Int. J. Food Microbiol. 208, 122–130. doi: 10.1016/j.ijfoodmicro.2015.06.001
Torriani, S., Felis, G. E., and Dellaglio, F. (2001). 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. 67, 3450–4345. doi: 10.1128/AEM.67.8.3450-3454.2001
Ventura, M., Canchaya, C., Meylan, V., Klaenhammer, T. R., and Zink, R. (2003). Analysis, characterization, and loci of the tuf genes in lactobacillus and bifidobacterium species and their direct application for species identification. Appl. Environ. Microbiol. 69, 6908–6922. doi: 10.1128/AEM.69.11.6908-6922.2003
Versalovic, J., Schneider, M., De Bruijn, F. J., and Lupski, J. R. (1994). Genomic fingerprinting of bacteria using repetitive sequence-based polymerase chain reaction. Methods Mol. Cell. Biol. 5, 25–40.
World Health Organization (WHO) (2012). Sodium Intake for Adults and Children. Available online at: http://www.who.int/nutrition/publications/guidelines/sodium_intake/en/
Keywords: NaCl reduction, microbial debittering, starter cultures, healthy olives, molecular approach
Citation: Pino A, Vaccalluzzo A, Solieri L, Romeo FV, Todaro A, Caggia C, Arroyo-López FN, Bautista-Gallego J and Randazzo CL (2019) Effect of Sequential Inoculum of Beta-Glucosidase Positive and Probiotic Strains on Brine Fermentation to Obtain Low Salt Sicilian Table Olives. Front. Microbiol. 10:174. doi: 10.3389/fmicb.2019.00174
Received: 30 October 2018; Accepted: 22 January 2019;
Published: 08 February 2019.
Edited by:Rosalba Lanciotti, University of Bologna, Italy
Reviewed by:Aldo Corsetti, Università Degli Studi di Teramo, Italy
Gianluca Bleve, Consiglio Nazionale Delle Ricerche, Italy
Copyright © 2019 Pino, Vaccalluzzo, Solieri, Romeo, Todaro, Caggia, Arroyo-López, Bautista-Gallego and Randazzo. This is an open-access article distributed under the terms of the Creative Commons Attribution License (CC BY). The use, distribution or reproduction in other forums is permitted, provided the original author(s) and the copyright owner(s) are credited and that the original publication in this journal is cited, in accordance with accepted academic practice. No use, distribution or reproduction is permitted which does not comply with these terms.
*Correspondence: Cinzia L. Randazzo, email@example.com