http://orcid.org/0000-0002-2786-6504
Figures
Abstract
Five different species of selected broad-spectrum antibiotic lactic acid bacteria isolated from extremely high–cold areas were used as starters to ferment indigenous forage oats and wheatgrass under rigid alpine climatic conditions. The five isolates were Lactobacillus plantarum QZ227, Enterococcus mundtii QZ251, Pediococcus cellicola QZ311, Leuconostoc mesenteroides QZ1137 and Lactococcus lactis QZ613, and commercial Lactobacillus plantarum FG1 was used as the positive control and sterile water as the negative control. The minimum and maximum temperatures were −22°C and 23°C during the fermentation process, respectively. The pH of wheatgrass silage fermented by the QZ227 and FG1 inocula reached the expected values (≤4.15) although the pathogens detected in the silage should be further investigated. All of the inocula additives used in this study were effective in improving the fermentation quality of oat silage as indicated by the higher content of lactic acid, lower pH values (≤4.17) and significant inhibition of pathogens. QZ227 exhibited a fermentation ability that was comparable with the commercial inoculum FG1 for the whole process, and the deterioration rate was significantly lower than for FG1 after storage for 7 months. The pathogens Escherichia coli, mold and yeast were counted and isolated from the deteriorated silage. E. coli were the main NH3-N producer while F. fungi and yeast produced very little.
Citation: Zhang M, Wang X, Cui M, Wang Y, Jiao Z, Tan Z (2018) Ensilage of oats and wheatgrass under natural alpine climatic conditions by indigenous lactic acid bacteria species isolated from high-cold areas. PLoS ONE 13(2): e0192368. https://doi.org/10.1371/journal.pone.0192368
Editor: Zhi Zhou, Purdue University, UNITED STATES
Received: July 18, 2017; Accepted: January 21, 2018; Published: February 6, 2018
Copyright: © 2018 Zhang et al. This is an open access article distributed under the terms of the Creative Commons Attribution License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original author and source are credited.
Data Availability: All relevant data are within the paper and its Supporting Information files.
Funding: This work was supported by the National Natural Science Foundation of China (Grant No. 41101244 to ZFT), a grant (No. 152300410037) from Henan Province of China. The funders had no role in study design, data collection and analysis, decision to publish, or preparation of the manuscript.
Competing interests: The authors have declared that no competing interests exist.
Introduction
Alpine grasslands on plateaus are sensitive and vulnerable to climate change and human disturbances [1]. A large number of livestock are slaughtered before winter due to the feed shortage caused by the harsh climate of these plateaus, the short frost-free period and the long grass withering period of at least 7 months from late September to May the following year [2]. Preservation and storage of feedstock material for continuous feeding of the ruminants throughout the year is a particular requirement in alpine regions [3].
Oats are the annual forage crop and are planted for green forage harvest in alpine regions to relieve stocking pressure on the grassland. Shepherds maintain the tradition of planting oats in alpine meadows all of the time. Wheatgrass is the common perennial pasture grass. Ensiling is an effective pretreatment technology for harvested crops that creates an acidic environment, which reduces the risk of feedstock decay and combustion under anaerobic conditions during later autumn and winter. However, fermentation of the silages is limited under low-temperature conditions, as not enough lactic acid is produced to improve the silage quality [4, 5]. The use of silage technology in alpine–cold plateaus is rather practical but rarely reported in previous studies.
Lactic acid bacteria (LAB) are able to be used as silage additives to ensure fast and vigorous fermentation because of their rapid accumulation of lactic acid and lower pH values at earlier stages of ensiling. The silage incubation temperature affects the species diversity of the LAB population with notable differences along a temperature gradient [4]. Their vulnerability to harsh environmental factors during the fermentation process remains a major challenge. The Tibetan plateau, being an average of 4 km above sea level makes it peculiarly cold for its latitude-colder than anywhere else outside the polar regions [6, 7]. The characteristics of the plateau environment, including low oxygen, low pressure, low average temperature, strong ultraviolet exposure and frequent disturbances, have a significant impact on microbial community and related functional genes [8, 9], and might lead to a distinctive LAB community. In our previous work, more than 2000 strains of LAB were isolated from plants, saline–alkali soil, a brine lake, indigenous yogurt, intestines of Gymnocypris przewalskii, etc. in the Qinghai–Tibet Plateau at an altitude of 3100 to 4800 m [1, 10], five of which were selected for use in this study because of their tolerance to acid, alkali, low and high temperature stress and inhibition of pathogens e.g. Micrococcus luteus, Escherichia coli, Staphylococcus aureus, Salmonella enterica, Listeria monocytogenes, Pseudomonas aeruginosa, and Bacillus subtilis.
Lactobacillus plantarum has been reported to be the most commonly used additive in silage fermentation, while the other LAB species have also been selected as silage inoculants because of their faster growth at high pH values than L. plantarum [11]. Previous studies have demonstrated that the promising effects of homo-fermentative or facultative hetero-fermentative LAB inoculation improve silage fermentation. Meanwhile, hetero-fermentative Lactobacillus buchneri and relatives such as Lactobacillus parabuchneri are able to degrade lactic acid to acetic acid with the concomitant production of 1,2-propanediol as well as traces of ethanol under anoxic conditions; however, they still improved the aerobic stability of silage [12–14].
Higher concentrations of NH3-N have been negatively associated with feedstock intake because they reduce ruminal motility and affect palatability [15, 16]. Low NH3-N content is an essential characteristic of well fermented silage. NH3-N is produced by the microbiota via urea degradation and amino acid deamination [17], but it is not conclusively known which microbiological species contribute the most to this process. We presume that different pathogens produce different amounts of NH3-N. In the present study, five broad-spectrum antibiotic isolates with stress resistance were selected to ferment silage under conditions that are typical of an alpine climate, and the homo-fermentative Pediococcus cellicola and hetero-fermentative Leuconostoc mesenteroides were used as compound starters. Our objective was to evaluate the effects of inoculation of LAB isolated from the plateau on the silage quality and prolongation of the preservation time of forage grass in alpine regions.
Materials and methods
Characteristics of the inocula
The sources of strains used as additives are shown in Table 1: QZ227 (L. plantarum) from wheat landrace, QZ251 (Enterococcus mundtii) from wild wheat, QZ311 (P. cellicola) and QZ1137 (L. mesenteroides) from wheatgrass and QZ613 (Lactococcus lactis) from bulrush were all isolated from a plateau located 3100 m above sea level in the Qinghai Plateau, China. The permission of the sampling location was issued by Zhengzhou University and the local farmers. Additionally, FG1 (L. plantarum, Snow Brand Seed Co. Ltd., Sapporo, Japan) was a commercial strain used as the positive control and sterile water was the negative control.
Morphological, physiological and biochemical tests were performed on the LAB isolates [18]. The abilities of LAB to resist salt, acid, alkali and low- and high-temperature stress were measured in reference to the methods of Ni et al. [19]. The growth rates of bacteria were assayed using the turbidimetry method at 600 nm combined with visual turbidity, with a sterile culture medium as the control. The antimicrobial activities of LAB isolates were detected by the agar diffusion method [20, 21]. Standard bacterial strains were all purchased from China General Microbiological Culture Collection Center (CGMCC), including M. luteus, E. coli, S. aureus, S. enterica, L. monocytogenes, P. aeruginosa and B. subtilis. Standard bacterial strains were inoculated on nutrient agar (NA, Qindao Hopebio Co. Ltd., Qingdao, China) at 30°C for 48 h in an electric thermostatted incubator (DNP-9022, Shanghai Jing Hong Laboratory Instrument Co., Ltd., Shanghai, China). Each single colony was adjusted to an optical density of 1.0 at 600 nm with sterile water, then the pathogen liquid was mixed with 5 ml of NA at 5°C to be used as the upper medium with NA as the lower medium. LAB isolates incubated at 30°C for 48 h in an anaerobic workstation (mini MACS, Don Whitley Scientific Ltd., West Yorkshire, UK) were centrifuged at 4500 g for 10 min. The supernatant was added to an Oxford cup (6 mm ×10 mm ×8 mm, Beijing Propbs Biotechnology Co., Ltd, Beijing, China) on double-medium. After anaerobic incubation at 30°C for 24 h, the inhibition zone diameter was measured using a Vernier caliper.
Silage preparation
Oats (Avena sative L. cv. Qinghai) were obtained as raw materials from an artificial forage grass farm at an elevation of 3100 m and wheatgrass (Agropyron trachycaulum cv. Endure) was obtained from a natural alpine pasture area at an elevation of 3300 m in Gonghe County, Hainan Tibetan Autonomous Prefecture, Qinghai Province, China. Oats (35 kg) and wheatgrass (35 kg) at the physical ripening stage above ground level were reaped in total to ensure no soil was included in mid-October 2015. Harvested oat and wheat materials were transported to a laboratory environment within 2 h. The whole of the wheatgrass and oat crops were chopped by hand to pieces of approximately 2 cm using scissors and sterilized with 75% alcohol. The revitalized LAB isolates were incubated in MRS broth (Lactobacillus agar as described by De Man, Rogosa and Sharpe; Merck, Darmstadt, Germany) for 24 h at 30°C. Each LAB inoculation (500 ml) was sprayed separately on 30 kg of feedstock and mixed thoroughly to reach a viable cell concentration of about 10 log10 CFU/g. Meanwhile, 250 ml of QZ311 inoculation and 250 ml of QZ1137 inoculation were blended to prepare the mixed fermenting agent, and 500 ml sterile water was the negative control. After thorough mixing, 200-g portions of the materials were repackaged in plastic film bags (Dragon N-6; Asahi Kasei Co., Tokyo, Japan), then degassed and sealed by a vacuum sealer (SQ-203S Vacuum Sealer; Asahi Kasei Co.). In total, 150 bags of each treatment were prepared and all of the ensiling bags (150 bags ×12 treatments arrangements) were placed outdoors on the plateau at 3100 m above sea level in Gonghe County, Qinghai Province, and local people were employed to guard them. The samples were collected in triplicate on days 1, 3, 7, 30 and 75 for analysis. Based on our research and experience of the color, smell, flavor and texture etc. of silage, combined with the sensory evaluation criteria of Ge et al.[22], quality assessment indicators are given. Classification was as follows: excellent, general, inferior. The remaining silage packages were used to determine the statistics of the deterioration rate at day 210.
Microbial community
The microbial community was counted by the dilution plating procedure. Samples of 10 g of silage material were shaken well with 90 ml of sterilized deionized water using a vortex mixer (IKA VORTEX 3, Staufen, Germany), and serial dilutions (10−1 to 10−5) were prepared in sterilized deionized water. Serial dilutions of 20 μl were spread on various agar medium plates (Nissui-Seiyaku Ltd., Tokyo, Japan). LAB were counted on MRS medium agar after incubation at 30°C for 48 h under anaerobic conditions. The aerobic bacteria were counted on NA, the yeasts and moulds were counted on potato dextrose agar (PDA) with a sterilized 10% dihydroxysuccinic acid solution (final concentration in total of 1.5%), and the E. coli were counted on blue light broth agar (BLB). NA, PDA and BLB agar media were purchased from QingDao Hopebio-Technology Co., Ltd, Qingdao, China. These agar plates were incubated at 30°C for 2 days. Moreover, 10−1 and 10−2 dilutions were spread on NA and Clostridium difficile agar for. B. subtilis and C. difficile, respectively, after heating in a water bath for 15 min at 75°C. The colonies were counted and the logarithmic numbers of viable colony-forming units in fresh matter (l g CFU/g FM) were calculated.
The numbered single colonies of E. coli, yeast and mold isolated in the deteriorated silage were amplified on their respective media and stored at −80°C for further testing of their ability to produce NH3-N. The pathogens were revitalized in NA liquid broth for 24 h, and the NH3-N content was measured with NA broth as the negative control and commercial counterparts (from the CGMCC) as the positive control.
Chemical composition
10 g of materials were shaken well with 90 ml of sterilized deionized water to determine the pH value via a glass electrode and pH meter (Mettler Toledo MP230; Greifensee, Switzerland), and then stored at −20°C before further NH3-N and organic acid analyses after being filtered with qualitative filter paper.
According to the official methods of the AOAC [23], dry matter, crude protein, and crude ash were assayed by the atmospheric pressure drying method (AOAC 934.01), the high temperature ashing method (AOAC 942.05), and the Kjeldahl method (AOAC 979.09), respectively. The remaining untreated silage was dried at 65°C for 48 h in an electro-thermostatic blast oven (Shanghai Shuli Instrument Co., Ltd., Shanghai, China), and the amount of dry matter was calculated according to the moisture losses. The dried silage was ground using a high-speed pulverizer (FW-100, Taisite Instrument Co., Ltd, Jinghai, Tianjin, China). The crude protein content of the silage powder was determined using an automatic Kjeldahl apparatus (K1100, Jinan Hanon instrument Co. Ltd., Jinan, China), with CuSO4 and K2SO4 at a ratio of 1:15 as the catalyst, and the standard concentration of the titrating H2SO4 solution was determined by sodium carbonate anhydrous with bromocresol green–methyl red mixed as the indicator. The crude ash content was calculated after incineration for 2 h at 550°C in a muffle furnace (REX-C900, RKC Instrument Inc., Osaka, Japan) and burning in an ashing furnace until no smoke was produced. The detergent fiber was determined by the Automatic Fiber Determination System (CXC-06, Zhejiang Top Instrument Ltd., Hangzhou, China).
The organic acid levels were measured by high performance liquid chromatography (column: Carbomix H-NP10: 8%, 7.8×300mm, Sepax Technologies, Inc., Delaware, USA; detector: DAD, 214nm, Waters 2695 instrument, Waters Co., Ltd., USA; eluent: 2.5mmol/L H2SO4, 0.6mL/min; temperature: 55°C). By calculating the relative retention times of certain peaks with lactic acid, acetic acid, propionic acid, butyric acid from Sigma company (Sigma Chemical Co. St. Louis, MO, USA) as the reference standards, the retention times for lactic acid, acetic acid, propionic acid and butyric acid were determined as 12.288 ± 0.011, 14.625 ± 0.014, 17.100 ± 0.003 and 20.964 ± 0.031 min, respectively.
NH3-N was measured with the indophenol blue method as described by Miao et al. [24]. Reagent A was prepared by dissolving 9.976 g phenol and 50.65 mg sodium nitroprusside in deionized water and diluting to 1l. Reagent B was prepared by dissolving 5 g NaOH and 13.5 ml NaClO successively in deionized water and diluting to 1l. Filtrate (2.0 ml) or distilled water (control) was placed in a tube and mixed with 8ml of 0.2 mol/l HCl, and 0.4 ml of the mixture was transferred to another tube and combined with 5 ml of reagent A and 5 ml of reagent B and incubated at 60°C for 10 min, cooled in cold water for 5 min, and the absorbance at 560 nm was measured by spectrophotometry using a TU1901 instrument (Beijing Purkinje General Instrument Co., Ltd., Beijing, China). A standard formula was created using a NH4Cl solution as the reference. The absorbance of the sample was then compared with the standard formula to determine the amount of NH4Cl using the following equation:
Statistical analyses
The experimental design was a randomized block due to the differences in time on the field before harvesting each batch of maize stalks for ensiling. Data were subjected to a two-way analysis of variance, with inocula and fermentation time as the main variables. Because significant interaction was seen for many variables, the effect of inocula was examined for each fermentation time by a one-way analysis of variance (ANOVA), followed by a multiple comparison by Tukey’s test. The statistical significance of antibacterial activity and the NH3-N producing ability of pathogens was evaluated with ANOVA with the Tukey's HSD test for post-hoc analysis. These analyses were carried out using IBM SPSS Statistics 19 procedure (https://www.ibm.com/analytics/cn). The pH variations and microbial community were plotted using Origin software Pro 8.5.1, (http://www.originlab.com/index.aspx?go=Products/Origin). A P-value of < 0.05 was considered statistically significant.
Results
The morphological, physiological and biochemical properties of five representative samples are shown in Table 2. The five isolates from Qinghai all grew well at low temperatures of 5°C–10°C, and survived at high temperatures of 45°C–50°C. All of the isolates grew well at 3.0% NaCl concentrations. All of the isolates survived at pH 3.0, and QZ227, QZ311, QZ1137 and QZ613 grew well at pH 3.5. QZ311, QZ1137 and QZ613 failed to survive at pH 10, while QZ227 grew weakly and QZ251 grew well under the same alkaline conditions. All of the isolates grew at pH 9.0.
The antibacterial activities of the bacteria are presented in Table 3. The selected LAB all showed broad-spectrum antibacterial activity and they had comparable levels of bacteriostatic ability, except that QZ227 displayed a stronger inhibiting effect on M. luteus than the commercial FG1 (P < 0.05) while QZ613 and QZ251 inhibited B. subtilis more strongly than FG1 (P < 0.05).
The moisture contents of the wheatgrass and oats were 51.12% and 62.20%, respectively. Small amounts of lactic acid and acetic acid were found in the pre-ensiled raw materials and LAB, F. fungi were found in wheatgrass at 1.48 and 2.98 log CFU/g, respectively, but not in oats (Table 4). According to our records and Weather China (www.weather.com.cn), the maximum and minimum temperatures ranged from −22°C to 23°C during the fermentation process from September 2014 to May 2015.
The quality assessment indicators are given in Table 5. The statistics of the deterioration rate at day 210 according to the distinguishing standard shown in Table 5: the excellent and general classes were counted as available silage and the inferior quality silages were counted as deteriorated.
The pH variations of the wheatgrass and oat silage are presented in Fig 1 and Table 6. During the process of fermentation, the pH of the negative control in the wheatgrass silages ranged from 5.66 to 6.45, while the pH of the control in oats ranged from 5.39 to 6.45. The pH of silages fermented by QZ227 and FG1 exhibited similar trends throughout the whole process. The pH values of wheatgrass and oat silages fermented by LAB exhibited the closest value on day 7. The pH of wheatgrass silage fermented by QZ227 decreased to its lowest value of 4.09 on day 30; meanwhile the pH values of wheatgrass silage fermented by QZ251, QZ311+1137 and QZ613 were all > 4.47 (Fig 1A, Table 6).
The pH of oat silage fermented by QZ227 reached a low value of 4.13 on day 7 (Fig 1B, Table 6). The pH of oat silages fermented by LAB decreased to < 4.30 on day 7 except for QZ613; however, the pH of the QZ613 treatment dropped to 4.24 on day 30 and continuously decreased to 4.17 at day 75, and the pH of oat silages with the other inoculations was reduced to below 4.16 on day 30 and remained below 4.13 at day 75.
B. subtilis was found on day 1 in both varieties of fermented silages, but its population was greatly reduced or had disappeared during the following fermentation process (Fig 2, Table 6). E. coli, F. fungi and yeast were detected in wheatgrass silage on day 1 (Fig 2A). On day 30, only QZ227 treated silage contained no pathogens, but E. coli, F. fungi and yeast were detected in it on day 75. E. coli were detected in oat silage of the control group throughout the whole process, although they were only detected in oat silage with bacteria on day 1 (Fig 2B). Small amounts of F. fungi were still detected in oat silage fermented by QZ227 and QZ251 on day 30.
The chemical composition of wheatgrass and oat silage fermented for 7, 30, and 75 days are shown in Table 6. Differences in inocula resulted in marked differences in fermentation products on day 7, while fermentation time also affected fermentation products. Propionic acid was only detected in control groups of wheatgrass silage on day 30. No butyric acid was found during the fermentation process, but the desired lactate and acetate accumulated (Table 6). On day 7, the lactate content of QZ227 reached 2.28 mg/g dry matter. The lactate contents of wheatgrass silages fermented by QZ227 and FG1 on days 1 and 3 were non-significant at P = 0.05, QZ227 exhibited the highest fermentation capacity of wheatgrass at 30 days with a lactate value of 7.96 mg/g DM, and was more effective for wheatgrass fermentation than FG1 at the earlier 30 days. Meanwhile, the oat silage fermented by QZ227 produced the most lactate on day 30 (12.74 ± 1.72mg/g DM), and the other additives reached their maximum contents on day 75. The lactate contents of oat silages fermented by QZ227 were similar to FG1 during first 7 days, but were significantly higher than FG1 at day 30 and 7 months (P < 0.05). The dry matter contents of the oat silages on day 75 were lower than those on day 30, while there were no significant differences between oat silages fermented by different additives. The NH3-N content of wheatgrass silage fermented by FG1 on day 30 was 1.21 ± 0.16 mg/g DM; moreover, the NH3-N contents of silages with inoculations were below 0.97 mg/g DM. Oats had higher lactate yields by day 75 when compared to wheat grass and that, oats also had higher protein content (Table 6).
The deterioration rates in total of both silages fermented for 7 months are shown in Table 7: no deteriorated silage samples of QZ227 were detected by the statistics, while the deterioration rate of FG1 was 2.38%. The deterioration rates of the rest of the silage samples with LAB additives were lower than that of the negative control group. As shown in Table 8, no Clostridium were detected in silages fermented for 7 months, while E. coli, mold and yeast were detected and isolated for further studies. The representative pathogens of E. coli isolated from the deteriorated silages produced NH3-N during the cultivation process, while the representative yeasts and molds produced little.
Discussion
The average environmental temperatures were low and the temperature differences were sharp during the fermentation process. LAB isolated from this extreme environment have a strong ability to adjust to the changing temperatures, and this may be helpful for silage making. In this study, the five isolates from the Qinghai Plateau were tolerant of acidic conditions and low temperatures, satisfying the demands for growth in low pH and low temperature environments.
The pH values and lactic acid and acetic acid concentrations were indicative of adequate fermentation of the silage [25]. The low pH achieved as a result of the accumulation of organic acids inhibited spoilage and pathogenic microbes, thereby preserving the nutritional contents of the ensiled forage [26]. In the present study, the pH of the wheatgrass silage fermented by FG1, QZ227, QZ311+1137 and QZ613 reached its lowest value on day 30 and increased slightly over the following days (Fig 1A), indicating the fermentation had reached a stationary phase on day 30. Meanwhile, the pH of wheatgrass silage fermented by QZ251 reached its lowest value on day 75 and then maintained a steady value. Similar pH trends were also found for oat silage. QZ251 exhibited a long fermenting time, but was effective. A previous study has shown that silages with pH values lower than 4.2 should be well preserved [27]. Only the pH of the wheatgrass silages fermented by QZ227 and commercial FG1 were in accordance with that criterion (Fig 1A). The pH of oat silages fermented by QZ227, QZ251 and QZ311+1137 were below 4.30 on day 7 (Fig 1B, Table 6), demonstrating that the three additive agents achieved the desired effect in oat silage by day 7. The pH of oat silage fermented by mixed QZ311+1137 was lower than that of QZ613 throughout the whole fermentation process (Fig 1B, Table 6), the lactate content was higher than that of QZ613 during the initial stages (Table 6), and the deterioration rate of QZ311+1137 was lower than that of QZ613 (Table 7). These results demonstrated that a mixed agent offers advantages over using a single starter. The lactate contents of oat silage fermented by QZ311+1137 were lower than that of QZ613 on days 30 and 75 (P<0.05). According to the study of Mansouri and Destain [28], the fermentation process is a kind of non-linear time-variant system, in which the control variables are closely interconnected, so that the phenomena observed in our study are normal but need further study.
There was a direct correlation between the pH value and the acid yield; the formation of lactate and acetate led to a decline in pH in this study. The main factors affecting the fermentation that have an impact on the proportion of produced organic acids are: the microbial population, inoculum source, substrate complexity, nutrient availability, pH, temperature and so on [29]. Our results shown that the fermentation time affects the silage of fermentation significantly, the acid yield decreased to a certain degree after the peak content had been reached, and this should be considered if long-term storage is needed. The results obtained from the present study indicate that oats and wheatgrass with selected bacteria can both be used as raw materials for silage; however, wheatgrass silage with bacteria is more suitable for short-term storage of less than 75 days because of its lowest pH and highest acetate contents on days 30. The five isolates displayed a broad antimicrobial spectrum against bacteria and fungi and could control pathogens during the ensiling process. Although the quality of wheatgrass silage with bacteria was significantly different compared to the negative control, the quality of wheatgrass silage was still barely satisfactory as the inhibition of pathogens in wheatgrass was limited. Wheatgrass fermented by QZ227 at 30 days could be recommended as a feedstock because of its few pathogens and high lactate contents.
The lactic acid-utilizing yeasts could simultaneously metabolize lactic acid as an energy source [30], and the major groups of strictly anaerobic bacteria use lactate as a common substrate [31]. F. fungi spoilage and related mycotoxin contamination in the metabolic products are some of the greatest risks of stored silage, which will eventually affect human health [3]. E. coli, B. bacillus, yeast and Clostridium were detected in oat silage on day 1, but had disappeared in oat silage fermented by FG1, QZ613 and QZ311+1137 on day 30. On day 75, no pathogens were detected in the oat silages with inoculations while large amounts of E. coli were always detected in the negative control group. The additive agent can effectively inhibit the pathogens during the fermentation process of oat silage.
The NH3-N contents of wheatgrass silage fermented by FG1 and QZ613 were high compared with the negative control wheatgrass on day 30 (Table 6); at this fermentation stage large amounts of E. coli were detected (Fig 2A). The NH3-N contents of the negative control oat silage were 1.09±0.54 on day 75 (Table 6); at this fermentation stage, E. coli were the only detected pathogens in the negative control group (Fig 2B). Combined with the results of Table 8, we concluded that the NH3-N contents of silages described previously were produced by E. coli although some other pathogens were detected.
The decisive factor affecting the silage nutritive value is the harvesting stage, and the fermentation process was reported to only have a slight impact on the nutritive value of maize silage [32]; this conclusion was verified partly in this study. The effects of different additives on the protein contents of silages were not significant; the fermentation time affected the dry matter significantly, the dry matter decreased with the fermentation time increased.
After storage for 7 months, silages fermented by QZ227 were well preserved, and silages fermented by FG1 were the next best preserved (Table 7). The other additives also decreased the probability of deterioration to some extent, with lower deterioration rates compared with the negative control group.
In conclusion, only FG1 and QZ227 could be used to ferment wheatgrass effectively on the plateau, while the other three agents played a fairly limited role. All of the inocula in this study could be used as additives to improve the fermentation quality of oat crops on the plateau.
Supporting information
S1 Fig. The variation in maximum and minimum temperature during the fermentation process from 092015 to 052016.
https://doi.org/10.1371/journal.pone.0192368.s001
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S1 Table. The pH variations of wheatgrass and oat silage.
https://doi.org/10.1371/journal.pone.0192368.s002
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S2 Table. The count of viable microorganism cells in oat silage at 1, 30 and 75 days.
https://doi.org/10.1371/journal.pone.0192368.s003
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S3 Table. The count of viable microorganism cells in wheatgrass silage at 1, 30 and 75 days.
https://doi.org/10.1371/journal.pone.0192368.s004
(DOC)
Acknowledgments
This work was supported by the National Natural Science Foundation of China (Grant No. 41101244), a grant (No. 152300410037) from Henan Province of China.
References
- 1.
Li Y. Lactic Acid Bacteria Resource Screening From the Tibet Plateau and Preliminary Research of Application [Master]: Zhengzhou University; 2013.
- 2. Zhang M, Lv HX, Tan ZF, Li Y, Wang YP, Pang HL, et al. Improving the fermentation quality of wheat straw silage stored at low temperature by psychrotrophic lactic acid bacteria. Animal Science Journal. 2017;88(2):277–85. PubMed PMID: WOS:000394664200010. pmid:27229440
- 3. Alonso VA, Pereyra CM, Keller LA, Dalcero AM, Rosa CA, Chiacchiera SM, et al. Fungi and mycotoxins in silage: an overview. Journal of Applied Microbiology. 2013;115(3):637–43. pmid:23445404
- 4. Zhou Y, Drouin P, Lafrenière C. Effect of temperature (5–25°C) on epiphytic lactic acid bacteria populations and fermentation of whole‐plant corn silage. Journal of Applied Microbiology. 2016;121(3):657. pmid:27271320
- 5. Cao Y, Cai Y, Hirakubo T, Fukui H, Matsuyama H. Fermentation characteristics and microorganism composition of total mixed ration silage with local food by-products in different seasons. Animal Science Journal. 2011;82(2):259–66. pmid:21729204
- 6. Qiu J. A sky-high view of the Third Pole: an interview with Tandong Yao and Weiming Fan. National Science Review. 2015;2(4):489–92. PubMed PMID: WOS:000367564100016.
- 7. Qiu J. China: The third pole. Nature. 2008;454:393–6. PubMed PMID: WOS:000257860300015. pmid:18650887
- 8. Johnson D, Campbell CD, Lee JA, Callaghan TV, Gwynnjones D. Arctic microorganisms respond more to elevated UV-B radiation than CO2. Nature. 2002;416(6876):82–3. pmid:11882896
- 9. Yang Y, Gao Y, Wang S, Xu D, Yu H, Wu L, et al. The microbial gene diversity along an elevation gradient of the Tibetan grassland. Isme Journal. 2014;8(2):430. pmid:23985745
- 10.
Lv H. Isolation, Identification and Preliminary Application Research of Lactic Acid Bacteria Resource in Animal Faeces and the Intestine of Gymnocypris przewalskii from the Tibet Plateau: Zhengzhou University; 2014.
- 11. Oliveira AS, Weinberg ZG, Ogunade IM, Cervantes AAP, Arriola KG, Jiang Y, et al. Meta-analysis of effects of inoculation with homofermentative and facultative heterofermentative lactic acid bacteria on silage fermentation, aerobic stability, and the performance of dairy cows. Journal of Dairy Science. 2017;100(6):4587–603. PubMed PMID: WOS:000401783800037. pmid:28342607
- 12. Driehuis F, Elferink SJWHO, Spoelstra SF. Anaerobic lactic acid degradation during ensilage of whole crop maize inoculated with Lactobacillus buchneri inhibits yeast growth and improves aerobic stability. Journal of Applied Microbiology. 1999;87(4):583–94. pmid:10583687
- 13. Elferink S, Krooneman J, Gottschal JC, Spoelstra SF, Faber F, Driehuis F. Anaerobic conversion of lactic acid to acetic acid and 1,2-propanediol by Lactobacillus buchneri. Appl Environ Microbiol. 2001;67(1):125–32. PubMed PMID: WOS:000166151300016. pmid:11133436
- 14. Wilkinson JM, Davies DR. The aerobic stability of silage: key findings and recent developments. Grass and Forage Science. 2013;68(1):1–19. PubMed PMID: WOS:000314476800001.
- 15. Li X, Xu W, Yang J, Zhao H, Pan C, Ding X, et al. Effects of applying lactic acid bacteria to the fermentation on a mixture of corn steep liquor and air-dried rice straw. Animal Nutrition. 2016;2(3):229–33. https://doi.org/10.1016/j.aninu.2016.04.003.
- 16. Oliveira AS, Weinberg ZG, Ogunade IM, Cervantes AA, Arriola KG, Jiang Y, et al. Meta-analysis of effects of inoculation with homofermentative and facultative heterofermentative lactic acid bacteria on silage fermentation, aerobic stability, and the performance of dairy cows. Journal of Dairy Science. 2017;100(6):4587–603. pmid:28342607
- 17. Kong X, Ji Y, Li H, Zhu Q, Blachier F, Geng M, et al. Colonic luminal microbiota and bacterial metabolite composition in pregnant Huanjiang mini-pigs: effects of food composition at different times of pregnancy. Scientific Reports. 2017;6:37224.
- 18. Xu Z, He H, Zhang S, Kong J. Effects of inoculants Lactobacillus brevis and Lactobacillus parafarraginis on the fermentation characteristics and microbial communities of corn stover silage. Scientific Reports. 2017;7(1):13614. pmid:29051616
- 19. Ni KK, Wang YP, Li DX, Cai YM, Pang HL. Characterization, Identification and Application of Lactic Acid Bacteria Isolated from Forage Paddy Rice Silage. Plos One. 2015;10(3):14. PubMed PMID: WOS:000353889600184. pmid:25803578
- 20. Coelho MC, Silva CCG, Ribeiro SC, Dapkevicius MLNE, Rosa HJD. Control of Listeria monocytogenes in fresh cheese using protective lactic acid bacteria. International Journal of Food Microbiology. 2014;191:53–9. pmid:25222327
- 21. Balouiri M, Sadiki M, Ibnsouda SK. Methods for in vitro evaluating antimicrobial activity: A review. Journal of Pharmaceutical Analysis. 2016;6(2):71–9. https://doi.org/10.1016/j.jpha.2015.11.005.
- 22. Ge J, Yang CJ, Liu GH. Nutritional evaluation of fresh and wilted mixed silage of naked oats (Avena nuda) and alfalfa (Medicago sativa). International Journal of Agriculture & Biology. 2015;17(4):761–6.
- 23.
AOAC. Official Methods of Analysis of AOAC INTERNATIONAL, 20th Edition2016.
- 24. Zhang M, Wang Y, Tan Z, Li Z, Li Y, Lv H, et al. Microorganism profile, fermentation quality and rumen digestibility in vitro of maize-stalk silages produced at different maturity stages. Crop and Pasture Science. 2017;68(3):225–33.
- 25. Menardo S, Balsari P, Tabacco E, Borreani G. Effect of conservation time and the addition of lactic acid bacteria on the biogas and methane production of corn stalk silage. BioEnergy Research. 2015;8(4):1810–23.
- 26. Ogunade IM, Kim DH, Jiang Y, Weinberg ZG, Jeong KC, Adesogan AT. Control of Escherichia coli O157:H7 in contaminated alfalfa silage: Effects of silage additives. Journal of Dairy Science. 2016;99(6):4427–36. PubMed PMID: WOS:000375876600031. pmid:27040788
- 27. Herrmann C, Idler C, Heiermann M. Improving aerobic stability and biogas production of maize silage using silage additives. Bioresource Technology. 2015;197:393–403. pmid:26348286
- 28. Mansouri M, Destain MF. An improved particle filtering for time-varying nonlinear prediction of biomass and grain protein content. Computers & Electronics in Agriculture. 2015;114(C):145–53.
- 29. Bastidas-Oyanedel JR, Bonk F, Thomsen MH, Schmidt JE. Dark fermentation biorefinery in the present and future (bio)chemical industry. Reviews in Environmental Science and Bio/Technology. 2015;14(3):473–98.
- 30. Kawahata M, Masaki K, Fujii T, Iefuji H. Yeast genes involved in response to lactic acid and acetic acid: acidic conditions caused by the organic acids in Saccharomyces cerevisiae cultures induce expression of intracellular metal metabolism genes regulated by Aft1p. Fems Yeast Research. 2006;6(6):924. pmid:16911514
- 31. Weghoff MC, Bertsch J, Müller V. A novel mode of lactate metabolism in strictly anaerobic bacteria. Environmental Microbiology. 2015;17(3):670. pmid:24762045
- 32. Loučka R, Hakl J, Jirmanová J, Tyrolová Y. Yearly variation in maize silage fermentation and nutritive quality. Grass & Forage Science. 2015;70(4):674–81.