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Review

Volatile Fatty Acids as Carbon Sources for Polyhydroxyalkanoates Production

by
Karolina Szacherska
1,
Piotr Oleskowicz-Popiel
2,
Slawomir Ciesielski
3 and
Justyna Mozejko-Ciesielska
1,*
1
Department of Microbiology and Mycology, Faculty of Biology and Biotechnology, University of Warmia and Mazury in Olsztyn, 10-719 Olsztyn, Poland
2
Water Supply and Bioeconomy Division, Faculty of Environmental Engineering and Energy, Poznan University of Technology, 60-965 Poznan, Poland
3
Department of Environmental Biotechnology, University of Warmia and Mazury in Olsztyn, 10-719 Olsztyn, Poland
*
Author to whom correspondence should be addressed.
Polymers 2021, 13(3), 321; https://doi.org/10.3390/polym13030321
Submission received: 1 December 2020 / Revised: 13 January 2021 / Accepted: 18 January 2021 / Published: 20 January 2021
(This article belongs to the Special Issue Production of Polyhydroxyalkanoate (PHA) Biopolymers from Waste Materials)
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Abstract

:
Waste of industrial origin produced from synthetic materials are a serious threat to the natural environment. The ending resources of fossil raw materials and increasingly restrictive legal standards for the management of plastic waste have led to research on the use of biopolymers, which, due to their properties, may be an ecological alternative to currently used petrochemical polymers. Polyhydroxyalkanoates (PHAs) have gained much attention in recent years as the next generation of environmentally friendly materials. Currently, a lot of research is being done to reduce the costs of the biological process of PHA synthesis, which is the main factor limiting the production of PHAs on the industrial scale. The volatile fatty acids (VFAs) produced by anaerobic digestion from organic industrial and food waste, and various types of wastewater could be suitable carbon sources for PHA production. Thus, reusing the organic waste, while reducing the future fossil fuel, originated from plastic waste. PHA production from VFAs seem to be a good approach since VFAs composition determines the constituents of PHAs polymer and is of great influence on its properties. In order to reduce the overall costs of PHA production to a more reasonable level, it will be necessary to design a bioprocess that maximizes VFAs production, which will be beneficial for the PHA synthesis. Additionally, a very important factor that affects the profitable production of PHAs from VFAs is the selection of a microbial producer that will effectively synthesize the desired bioproduct. PHA production from VFAs has gained significant interest since VFAs composition determines the constituents of PHA polymer. Thus far, the conversion of VFAs into PHAs using pure bacterial cultures has received little attention, and the majority of studies have used mixed microbial communities for this purpose. This review discusses the current state of knowledge on PHAs synthesized by microorganisms cultured on VFAs.

Graphical Abstract

1. Introduction

Nowadays, petroleum-based plastics, due to their properties, are one of the most common materials in modern society. Constant production of materials based on synthetic polymers and their intensive human overconsumption leads to irreversible changes that have a negative impact on the natural environment and human health. The growing accumulation of non-biodegradable polymer wastes and the exhaustive reserves of fossil fuels prompted scientists to develop new biopolymer production technologies. Biopolymers are gaining more interest due to not only their biodegradability/compostability, but also biocompatibility, and bio-based nature. Various types of biodegradable polymers are being used in various fields. They are grouped depending on their composition. Polymers like starch and cellulose belong to the first group and are produced from agro-resources. The second group includes biopolymers synthesized by microorganisms during microbial processes, e.g., polyhydroxyalkanoates (PHAs). The third group consists of polymers that are conventionally and chemically synthesized (polylactic acid (PLA)). The fourth group contains blends of renewable resources with synthetic monomers (soy-based urethanes) [1]. However, until now, PLA and PHAs are the key players in the market for biodegradable polymers. PLA has gained much attention as the effective polymer for biomedical and packing composites. Nonetheless, due to fragility, reduced impact strength, and low thermal stability, PLA has become a hurdle for the application in engineering purposes [2]. Additionally, PHAs are attracting attention as the next generation of environmentally friendly materials and have become an alternative to synthetic polymers because they are completely biodegradable, biocompatible and can be produced from renewable sources [3]. The worldwide production of PHAs from commercial manufacturers reached up to 2.05 million tons in 2017 [4]. The interest in renewable, eco-friendly, and bio-based materials is still high, suggesting that the biopolymers market will be a serious player in the future. It is predicted that the global market value of PHA will grow from USD 57 million in 2019 to USD 98 million by 2024 [5].
PHAs are water-insoluble biopolymers synthesized by microorganisms and collected intracellularly as granular supplementary substances. Microorganisms accumulate PHAs as a reserve material, serving as energy in the presence of excess carbon source and limited concentration of essential nutrients (nitrogen, phosphorus, magnesium, and oxygen) [6]. Excess carbon is used for cell growth and the PHA storage process, and after depletion of carbon source, the stored polymers are used by microorganisms as a source of carbon and energy. PHAs are synthesized by gram-negative bacteria and gram-positive ones, which belong to genera such as Pseudomonas, Bacillus, Cupriavidus, Aeromonas and Rhodobacter. Thus far, only a few species of bacteria have met the optimal PHA production criteria. The most important are Cupriavidus necator, Alcaligenes latus, Pseudomonas oleovorans or Pseudomonas putida. Microorganisms produce a number of PHAs differing in chemical structure. These polymers consist of 100 to 30,000 monomers that bind to each other with ester bonds. The type of the biopolymer synthesized depends on the carbon source, the PHA producer and the bioprocess conditions. Over 150 different types of PHAs are synthesized by various bacterial species under different growth conditions. PHAs are classified based on the number of carbon atoms present in the biopolymer molecule and they can be divided into short-chain-length (PHASCL), medium-chain-length (PHAMCL) and long-chain-length (PHALCL) PHAs. PHASCL contains from three to five carbon atoms, e.g., poly-3-hydroxybutyric acid and poly-3-hydroxyvaleric acid. PHASCL is rigid and brittle thermoplastic biopolymer with a high degree of crystallinity (60%–80%) [7]. This type of PHA can be produced by a single species (e.g., Cupriavidus necator) as well as by mixed microbial cultures (MMC) derived from activated sludge. These polymers can be used in industry in the production of containers and packaging for everyday use. They can be the subject of investigation as food packaging materials due to their processing possibility to packaging films via thermoforming, a high water vapor barrier, a high barrier properties against CO2, a high oxygen barrier hampered the growth of aerobic microbes and the oxidative spoilage of unsaturated fatty acids [8]. The low oxygen transmission rate and water and CO2 barriers make PHAs an interesting basic materials for producing bottles for liquid foods, and also for CO2-containing liquids [9]. As a major drawback of using PHAs as food packaging material is still not satisfying a cost-performance scenario mainly because of the high expenses of raw materials [10]. PHAMCL contain from 6 to 14 carbon atoms in the molecule, e.g., poly-3-hydroxyoctanoic acid or poly-3-hydroxydecanoic acid. They have elastomeric properties and are flexible biopolymers with low crystallinity, low tensile strength, high elongation to break, low melting point and glass transition (below room temperature). PHAMCL are mainly produced by bacteria of the genus Pseudomonas. Due to their properties, these polymers can be widely used in the production of paints and pigments, as well as in medicine and pharmacy. PHALCL contain more than 14 carbon atoms in their structure, e.g., poly-3-hydroxyhexadecanoic acid [11]. This type of biopolyester is uncommon and knowledge about its properties and potential applications is still limited.
The main limitation in the production of PHA on a large scale is the high process costs, which are 15 times higher than in the case of conventional plastics [10]. Furthermore, the productivity of PHA during fermentations in terms of the amount of PHA formed per liquid volume per time (g PHA/L/h) is an important factor for techno-economical evaluation of this bioprocess. Therefore, it seems reasonable to use substrates that will not only be effectively used by microorganisms for growth and PHA synthesis, but can be obtained at prices that will guarantee the profitability of the process. These substrates could be waste materials such as organic industrial and food waste, and various types of wastewater [12,13,14]. The use of wastes for the production of biopolymers is a beneficial approach, ensuring the disposal of harmful substances and the creation of environmentally friendly materials [15]. Particular attention has been given to volatile fatty acids (VFAs), which are generated by anaerobic fermentation, such as acetic acid, propionic acid, butyric acid, valeric acid and caproic acid [16,17]. Previous results have shown that VFAs could be effectively used by microorganisms as a source of carbon and energy for the growth and production of PHAs [12,18].
For producing VFAs via anaerobic digestion, the organic fraction of municipal solid waste (OFMSW) is a promising potential substrate. The ever-growing amount of food waste in Europe, reaching about 90 million tons per year, requires the development of innovative solutions to the processing and disposing of it [19]. Therefore, OFMSW is subjected to anaerobic digestion to produce and extract VFAs, which can be further used as valuable sources of carbon for the production of value-added PHAs. Valentino et al. [20] conducted OFMSW fermentation for VFAs production at 55 °C using a 200 L continuous stirred-tank reactor (CSTR) with a hydraulic retention time (HRT) of 3.3 d and an average organic loading rate (OLR) of 20 kg VS/m3·d. An acidic environment (pH 5.0–5.6) was maintained by recirculation of digestate from a parallel thermophilic anaerobic fermenter. VFA production reached its maximum (22.3 g CODVFA/L) on day 9 (2.7 HRTs). In the fermented VFA stream, butyric acid (37.2%), acetic acid (23.4%), propionic acid (13.2%), valeric acid (10.9%) and caproic acid (9.6%) predominated. The authors also found smaller amounts of isobutyric acid (3.56%) and isovaleric acid (1.44%). Furthermore, it has been shown that pH can influence the rate of VFA production. Cheah et al. [21] revealed that a pH of nine can lead to a higher production of VFAs (high in acetic acid) than a pH of six. They demonstrated that the concentration of VFAs in wastewater increased up to 11.5 g/L.
The aim of this review is to present the challenges to bacterial PHA production using VFAs. Knowledge about the use of VFAs to synthesize PHAs is currently limited, so this review focuses on systematizing their potential in this field.

2. Characterization and Production of Volatile Fatty Acids

VFAs are linear short-chain fatty acids containing from two (acetic acid) to six (caproic acid) carbon atoms. Table 1 presents the characteristics and properties of VFAs.
Recently, special attention has been paid to the production and recovery of VFAs due to their high potential as renewable carbon sources and their broad range of applications [24]. VFAs can be used as sources in the production of biopolymers or biofuels (methane and hydrogen) and in the biological removal of nutrients from wastewater [25,26,27]. Due to the fact that VFAs contain a carboxylic group, they are also used in conventional organic chemistry as precursors of reduced chemical compounds and derivatives (aldehydes, alcohols, alkanes, ketones or esters) [28].
VFAs are intermediate products in the process of anaerobic digestion (AD) of various types of waste, such as food waste, municipal waste, agricultural waste, milk sewage, paper and cellulose sewage. Many microorganisms were reported to be capable of generating VFAs, such as acetic acid, propionic acid and butyric acid using a variety of substrates (Table 2). The AD process consists of a series of stages in which the organic matter is degraded by microorganisms under anaerobic conditions [29]. The synthesis of VFAs by mixed microbial cultures (MMC) is possible due to various metabolic pathways that occur inside cells, depending on the substrate used.
In many cases, co-fermentation of different wastes was employed, for example, agricultural waste and animal manure [30], or waste activated sludge and corn straw [31]. The purpose of co-fermentation is to balance the C/N ratio. Some experiments showed that an increase in the C/N ratio supported the growth of microorganisms responsible for acidogenesis [32,33]. In order to increase the efficiency of VFA production by MMCs, special attention should be paid to the conditions and parameters of the process. In particular, different hydraulic retention times (HRT), organic loading rates (OLR), temperatures and pHs can affect the productivity of VFAs. It is also possible that other by-products will be formed, e.g., long-chain fatty acids, alcohols, biohydrogen, biomethane, esters and other intermediates [34,35].
Bermúdez-Penabad et al. [36] studied the effect of different pH values (from 5.0 to 10.0) on the AD of tuna waste to produce VFAs. The authors showed that varying the pH influenced the production of VFAs. After 32 days of digestion of tuna waste, the highest total VFAs concentration at pH 8 was 30.611 mg COD/L. The resulting VFAs consisted mainly of acetic acid, propionic acid, butyric acid and valeric acid. Furthermore, acetic acid was the dominant product at all pH values tested. Den Boer et al. [37] used a co-culture consisting of Klebsiella mobilis and Escherichia coli to produce short-chain and medium-chain VFAs from kitchen biowaste and potato peels. The authors tested the effects of various feeding strategies to increase chain elongation under microaerobic conditions at pH 6.0–6.5. In the initial stages of the process, acetic acid and ethanol dominated, while in the later stages, an accumulation of propionic acid was observed, followed by accumulation of butyric and valeric acid. The highest level of final products, 325 mg/g TS, was obtained at pH 6.5, with a yield of 448 mg/L/h. Moretto et al. [38] optimized the fermentation process of urban organic waste to produce a stream rich in VFAs. The effects of different temperatures, pH values, HRTs and OLRs were studied in both batch and continuous processes. Using batch processes at a temperature of 37 °C and a pH of 9 ensured the production of VFAs using waste feedstock thermally pretreated for 76 h at 72 °C. At a later stage, these conditions were used in a continuous process, resulting in the efficient production of VFAs with high levels of VFAs (0.77 CODVFA/VS(0) and 39 g CODVFA/L).
VFAs converted anaerobically from various waste streams could be a promising platform for PHA production. The process of PHA synthesis by microorganisms using waste-derived substrate required expensive enzymes, sterilization processes, and high energy demand, which increases the overall production cost. The synthesis of PHAs using low-cost materials, such as VFAs as the feedstock, is considered to be an economical approach. Furthermore, PHA production from VFAs seems to be a good approach since VFAs composition determines the constituents of PHA polymer and has a great influence on the properties of PHAs [39].
Table
Table 2. Production of volatile fatty acids by microorganisms.
Table 2. Production of volatile fatty acids by microorganisms.
Volatile Fatty AcidBacteriaSubstrateConcentration (g/L)Productivity (g/L/h)References
Acetic acidAcetobacter aceticheese whey96.94.060[40]
Clostridium acetiummixed gas (4% H2:18% Argon:78% CO)1.3nd[41]
Clostridium lentocellum SG6paddy straw30.9nd[42]
Moorella thermoaceticasugarcane straw hydrolysate17.2nd[43]
Saccharomyces cerevisiae + Acetobacter pasteurianusglucose66.00.367[44]
Propionic acidPropionibacterium acidipropionici (ATCC 4965)lactate15.10.113[45]
glycerol6.80.051
sugarcane molasses8.20.062
Propionibacterium acidipropionici (CGMCC 1.223)glycerol44.60.200[46]
Propionibacterium acidipropionici (ATCC 4875)hemicellulose hydrolysate18.0nd[47]
chesse whey19.70.980[48]
Propionibacterium freudenreichii CCTCC M207015glucose67.10.140[49]
Propionibacterium freudenreichii spp. shermaniiglycerol9.00.180[50]
Butyric acidClostridium butyricum S21sucrose20.00.210[51]
Clostridium butyricum ZJUCBglucose16.7nd[52]
Clostridium thermobutyricum JW171Kglucose18.42.400[53]
Clostridium tyrobutyricumcorn husk hydrolysate20.80.420[54]
sugarcane bagasse hydrolysate20.90.510[55]
nd—not determine.

3. Synthesis of PHAs from VFAs by Pure Bacterial Cultures

In order to launch PHAs into the market, there is a need to reduce the costs involved in the production of these biopolymers. Therefore, the use of cheap substrates, including VFAs, may contribute to lowering the cost of obtaining the final bioproduct [56]. Numerous metabolic pathways are involved in VFA synthesis. VFAs are also the preferred carbon source for the synthesis of PHAs, because they are direct metabolic precursors in the PHA biosynthesis pathway (Figure 1). Several pure bacterial cultures are capable of producing PHAs in satisfactory amounts using VFAs as substrates (Table 3).
Poly(3-hydroxybutyrate) [(P(3HB)] is the most well-known and the most widely studied polyhydroxyalkanoic acid. It is a brittle biopolymer with low elasticity, high O2 barrier, good thermoplastic properties and poor mechanical properties [67]. Chakraborty et al. [57] investigated the ability of Ralstonia eutropha ATCC 17699 to produce PHAs using acetic, propionic and butyric acid. This strain synthesizes homopolymer P(3HB) at a concentration of about 31% of cell dry weight (CDW) using acetic and butyric acid. However, higher productivity (0.037 g PHA/g substrate) was observed in a cultivation supplemented with butyric acid. According to López et al. [18], Methylocystis hirsuta was able to produce up to 52% of the CDW when grown on acetic and butyric acid as co-substrates during artificial biogas-based cultivation under nitrogen limiting conditions. Higher P(3HB) content was revealed in Bacillus megaterium OU303A isolated from municipal sewage sludge [58]. The authors found that this strain synthesized 62.43% of CDW in the presence of propionic acid in a medium containing glycerol. A slightly lower concentration (58.63% of CDW) was observed when the growth medium was supplemented with glucose. The obtained data suggested that the addition of propionic acid supported PHAs synthesis. The bacteria accumulated higher amounts of PHAs when this VFA was added, as compared to the use of individual carbon sources (glucose and glycerol). However, a two times lower P(3HB) content was reached with Bacillus sp. INT005 cells cultured on butyric acid [64].
In addition to homopolymers, pure bacterial cultures are able to biosynthesize copolymers using VFAs as carbon sources. Studies have shown that incorporating other PHA monomers into P(3HB) will significantly improve the mechanical properties of a final product, reduce crystallinity and melting temperature, and increase flexibility [68]. Kumar et al. [69] reported that bacteria belonging to the Bacillus genus are capable of synthesizing copolymers during cultivations supplemented with a specific mixture of VFAs obtained through the controlled hydrolysis of various wastes, such as pea shells, apple pomace, onion peels, and potato peels. The authors found that Bacillus thuringiensis EGU45 and Bacillus cereus EGU43 cultured on pea shells hydrolysates accumulated P(3HB-co-3HV) copolymer with a 3HV content of 1% w/w. Furthermore, it was observed that the efficiency of PHA synthesis could be improved by the addition of onion peel hydrolysate together with the supplementation with glucose. Interestingly, VFAs were not detected after the PHA production phase, suggesting that the applied waste hydrolysates supported efficient bacterial growth, and biopolyester synthesis and accumulation. Furthermore, the effect of combining cultures on PHA production was evaluated by Munir and Jamil [59]. The authors confirmed that a co-culture of Pseudomonas sp. ST2 and Bacillus sp. CS8 was capable of producing up to 35% P(3HB-co-3HV) copolymer when grown on acetic and propionic acids in combination with glucose. When a glucose and propionic acid mixture was used as a feedstock, the individual strains produced more PHAs than with glucose as the only carbon source. Furthermore, it was observed that Alcaligenes eutrophus NCIMB 11599 produced a higher P(3HB-co-3HV) copolymer yield and 3HV fraction of the copolymer in a two-stage fed-batch cultivation when using valeric acid than when using propionic acid. Additionally, Ralstonia eutropha KCTC 2658 has been identified as a PHAs copolymer producer when cultured on a mixture of acetic, propionic, and butyric acid [61]. It was reported that P(3HB-co-3HV) production reached 50% CDW using 5 g/L of acetic-acid:propionic-acid:butyric-acid at a proportion of 1:2:2. Furthermore, the authors confirmed that the applied conditions enabled the production of biopolyesters with a 3HV molar fraction of 21 mol%. Interestingly, Ralstonia eutropha ATCC 17699 synthesized the copolymer with a higher 3HV fraction (35 mol%), but the cell dry weight and biopolymers content in cells were lower (1.2 g/L and 25% of CDW, respectively). In addition, it was observed that the proportion of VFAs to co-substrates has an influence on the biomass, PHAs content and biopolymer composition. According to Du et al. [63], a low ratio of propionic acid to glucose led to a low concentration of 3HV fraction, but high dry cell weight and P(3HB-co-3HV) productivity. In contrast, a high propionic-acid-to-glucose ratio led to a high 3HV concentration but a low P(3HB-co-3HV) content in Ralstonia eutropha cells.
In addition, Jeon et al. [70] determined that, by altering the levels of the acetyl-CoA pool, it is possible to improve the concentration of 3HV in P(3HB-co-3HV). They overexpressed acetyl-CoA acetyltransferase (atoAD) in a recombinant Escherichia coli YH090 carrying genes responsible for PHA synthesis (bktB, phaB, and phaC). Use of propionic acid as a carbon source stimulated copolymer synthesis, resulting in a 7.3-fold higher 3HV fraction (67.9 mol%) in the copolymer produced by the above-mentioned mutant than by the strain without the overexpression of atoAD genes. Further, Hydrogenophaga pseudoflava grown in a medium supplemented with non-hydrolyzed lactose whey and valeric acid was able to synthesize up to 40% P(3HB-co-3HV) with 5 mol% 3HV [71].
A substantial amount of P(3HB-co-3HV) copolymer (55% of CDW) was synthesized by Cupriavidus necator cultured on olive mill wastewater effluent rich in acetic, propionic and butyric acid (OMWAcid) without adding any exogenous substrate. OMWAcid contained not only different short chain VFAs, but also polyphenols (1.2 g/L), N-NH4 (60 mg/L), proteins (1.56 g/L), and lipids (3.24 g/L). Furthermore, it was observed that OMWAcid at concentrations of 75% and 100% inhibited the synthesis and accumulation of the copolymer. This work shows that residues from the fermentation of wastes can be used for the biosynthesis of bacterial biopolymers [62]. Such approaches can potentially reduce the production costs of PHAs and offer environmental benefits through the reuse of wastes. It was demonstrated that the type II methanotroph Methylocystis hirsuta is capable of synthesizing P(3HB-co-3HV) copolymer using artificial biogas with the addition of VFAs [18]. The highest copolymer concentration was observed in a cultivation with valeric acid as a co-substrate (53.8% of CDW), and the highest 3-hydroxyvalerate content (13.5%) was found within the biocomposite. The same strain accumulated trace amounts of these biopolymers using pure VFAs as the only carbon sources (from 1.1 to 9.0% of CDW). Recently, Ferre-Guell and Winterburn [60] obtained increased P(3HB-co-3HV) copolymer concentrations in a cultivation of Haloferax mediterranei grown on a mixture of butyrate and valerate acids with the addition of surfactants to increase substrate bioavailability. The studied strain was able to synthesize up to 59% of the copolymer, resulting in a productivity rate of 10.2 mg/L/h in the fed-batch fermentation. These results demonstrate that a VFA mixture with the addition of Tween 80 supports the synthesis of polymers containing the desired 3HV fraction of 43 mol%.
Thus far, only one study reported the production of mcl-PHAs using VFAs. Cerrone et al. [66] studied the effect of nitrogen limitation on the growth, and synthesis and accumulation of mcl-PHAs by three Pseudomonas putida strains (KT2440, CA-3 and GO16) using VFAs produced from the anaerobic digestion of a lignocellulosic substrate. The effluent that was used as a carbon source to support growth and mcl-PHA synthesis consisted of 15.3 g/L of VFAs (from acetic acid to valeric acid) with a predominance of butyric acid (12.8 g/L). The results revealed that the analyzed strains differed in their ability to grow and accumulate mcl-PHAs. The highest mcl-PHA concentration (44% CDW) was detected in the cells of Pseudomonas putida KT2440 cultured on butyric acid and acetic acid. Similar levels of biopolyesters were extracted from Pseudomonas putida CA-3 grown on acetic, propionic or butyric acid. Furthermore, the production of mcl-PHAs was lower with the GO16 strain than with the KT2440 and CA-3 strains, regardless of the type of VFA. However, gas chromatography analysis revealed that the monomeric composition of the mcl-PHAs extracted from P. putida KT2440 and CA-3 cells was similar. The authors reported that 3-hydroxydecanoic acid (3-HD) was the major component. Furthermore, this biopolyester was found to contain lesser amounts of 3-hydroxyoctanoic acid (3-HO) and 3-hydroxydodecanoic acid (3-HDD), and trace amounts of 3-hydroxytetradecanoic acid (3-HTD). Interestingly, Pseudomonas putida GO16 produced mcl-PHAs containing higher levels of 3-HDD monomer than those produced by the KT2440 and CA-3 strains, suggesting that its level is dependent on bacterial strain.

4. Synthesis of PHAs from VFAs by Mixed Microbial Cultures

Recently, interest in using MMC for the production of PHAs has increased significantly among researchers. MMC are communities of microorganisms that have the ability to cooperate with each other by carrying out specific intracellular and extracellular reactions. The process of using MMC for the synthesis of PHAs can be economically competitive with the production of PHAs by pure bacterial cultures [72]. Using mixed cultures is simpler and requires less investment and operational expenses in terms of sterile conditions and a feedstock preparation. VFAs such as acetate, propionate, butyrate and valerate can be used efficiently by mixed microbial cultures for the synthesis of PHAs (Table 4).
Acetic acid is one of the best-studied carbon sources for the synthesis of PHAs by mixed cultures under feast and famine conditions. In the metabolic pathway, acetic acid is transformed into P(3HB). The efficiency and rate of polymer synthesis depend on the operating conditions of the bioreactor. Serafim et al. [73] found that aerobic dynamic substrate feeding (ADF) in a sequencing batch reactor (SBR) operated under ammonia limitation favored the selection of cultures with a high P(3HB) storage capacity. Furthermore, the authors observed that the P(3HB) specific storage rate could have been inhibited due to the acetic acid concentration. They confirmed that P(3HB) content reached 67.5% when acetic acid was supplied in one pulse at a concentration of 180 Cmmol/L. However, feeding the substrate pulse-wise caused an increase in the P(3HB) storage rate (78.5%). Beun et al. [74] reported that, during the feast period in an SBR reactor, the P(3HB) content reached only 40% CDW. It was also shown that, in the subsequent fed-batch, the enriched mixed culture was able to produce up to 89% CDW within 7.6 h of continuous feeding with acetic acid [75]. Furthermore, it was concluded that, the longer the cultivation in the feast-famine SBR, the higher the P(3HB) production rate. The average specific rate of PHB production over the first 7.6 h was 1.4 C-mol/C-mol/h (1.2 g/g/h). Moreover, it was proved that the presence of acetic acid stimulates the consumption of butyrate and propionate due to the reactivation of acetyl-CoA, and thus supports the internal activity of cellular metabolism. Thus, it can be assumed that acetic acid is one of the most appreciated VFAs in the production of PHAs by microorganisms [76].
Table
Table 4. Production of PHAs by mixed microbial cultures using volatile fatty acids.
Table 4. Production of PHAs by mixed microbial cultures using volatile fatty acids.
Carbon SourceType of PHAPHA (%) References
Acetic acidP(3HB)40.0[74]
P(3HB)78.5[73]
P(3HB)89.0[75]
Municipal wastewater + acetic acidP(3HB)30.0[77]
Fermented paper mill wastewater (acetic acid, propionic acid, butyric acid, valeric acid)P(3HB-co-3HV)48.0[78]
Fermented molasses (acetic acid, propionic acid, butyric acid, valeric acid)P(3HB-co-3HV)66.0[14]
Fermented food waste (acetic acid, propionic acid, butyric acid, valeric acid) + dewatered sludgeP(3HB-co-3HV)64.5[79]
Fermented paperboard mill wastewater (acetic acid, propionic acid, butyric acid, valeric acid)P(3HB-co-3HV)67.4[80]
Sludge hydrolysis liquid (acetic acid, propionic acid, butyric acid, valeric acid)P(3HB-co-3HV)24.1[81]
Fermented crude glycerol P(3HB-co-3HV)76.0[82]
Fermented wood waste (acetic acid, propionic acid, butyric acid)P(3HB-co-3HV)50.3[83]
Fermented cheese whey (acetic acid, propionic acid, butyric acid, valeric acid)P(3HB-co-3HV)30.0[84]
The substrate composition seems to be an important factor that strongly affects the diversity of PHA monomers. Fradinho et al. [76] evaluated the feeding of an acetate-enriched photosynthetic mixed culture (PMC) with mixed VFAs. The authors showed that acetic acid and butyric acid supported P(3HB) homopolymer synthesis, whereas propionic acid supported the formation of P(3HB-co-3HV) copolymers consisting of 51% 3HV. Furthermore, a low acetate concentration (<30 CmM) and specific light intensities around 20 W/gX were determined to be the optimal operating conditions that enable the improvement of P(3HB-co-3HV) content from 15% to 30% in less than 4 h [74]. Additionally, Lemos et al. [85] confirmed that, by manipulating the feed VFA profiles, polymers with different monomer compositions could be synthesized. The results indicated that sludge fed with acetate was able to produce a P(3HB) homopolymer, whereas sludge fed with propionate was capable of synthesizing a P(3HB-co-3HV) copolymer. Furthermore, switching the substrate feeds, i.e., feeding propionic acid to sludge adapted to acetate and acetic acid to sludge adapted to propionate, led to the production of a P(3HB-co-3HV-3HMV) terpolymer.
In the field of PHA biosynthesis, attention has focused on the possibility of using pretreated sludge as a possible carbon source for the synthesis of these polymers. Liao et al. [81] demonstrated that VFAs from heat-pretreated sludge hydrolyzed liquid could support PHA synthesis and accumulation. The authors observed that different heat pretreatment temperatures affect the composition of VFAs, and consequently, the biopolymer productivity rate. Hydrolyzed liquid that was heat pretreated at 60 °C was the optimal carbon source for P(3HB-co-3HV) synthesis, and the maximal copolymer content was 24.1% CDW. At that temperature, acetic acid was the predominant VFA in the hydrolyzed liquid, whereas propionic, butyric and valeric acid were present in smaller amounts. Chua et al. [77] noted that sludge acclimatized with municipal wastewater supplemented with acetic acid could accumulate PHAs up to 30% CDW, whereas sludge without this VFA accumulated 20% CDW.
Wastewater from waste-glycerol fermentation supplemented with different amounts of acetic and propionic acids improves PHA production capacity. In an SBR reactor, a mixed microbial community fed a substrate of organic acids supplemented with acetic acid produced P(3HB), while propionic acid supported P(3HB-co-3HV) synthesis. Genetic analysis revealed that Thauera sp. predominated in the reactor with acetate, while Paracoccus denitrificans predominated in the reactor with propionate [86]. Additionally, Burniol-Figols et al. [82], using fermented crude glycerol and mixed microbial consortia, confirmed the possibility of selectively converting VFAs into PHAs. The authors extracted up to 76% P(3HB-co-HV) from an SBR reactor where the dominant bacterial taxa were Amaricoccus and Thauera, which accounted for 56.3%–72.4% of the whole microbial community.
Chen et al. [79] showed the effect of VFAs obtained from co-fermentation of municipal wastewater and food waste on the production of PHAs, and revealed that the feeding regimes affect the rate of PHA synthesis. Continuous pulsed feeding with fermentation fluid containing VFAs (acetic acid, propionic acid, butyric acid, and valeric acid) was most effective, leading to the highest P(3HB-co-3HV) synthesis rate of 64.5%. A similar copolymer content (66% of CDW) was observed when mixed cultures were supplemented with VFAs from fermented molasses [14]. The use of a continuous feeding strategy seems to be more efficient than a pulse feeding strategy and results in higher biopolymer productivity. Furthermore, a continuous feeding regime increased the 3HV content by 8% compared to one using pulse-wise feeding. Lower copolymer content (50.3% of CDW) was observed by Li et al. [83] when VFAs obtained from the co-fermentation of pretreated wood waste and sewage were used as a feedstock. The authors showed that the PHA production rate reached 0.237 g COD PHA/L/h. Monomeric composition analysis revealed that mixed microbial consortia were able to produce P(3HB-co-3HV) copolymer that contained only the 6 mol% 3HV fraction. Promising results were described by Bengtsson et al. [78], who demonstrated that activated sludge cultivated on VFAs produced by acidogenic fermentation of paper mill wastewater was capable of synthesizing 48% CDW of P(3HB-co-3HV). A higher PHA content was obtained using acetate-enriched bacteria growing on the same fermented effluent [80]. The final biopolymer content was 58.57%, while the PHA yield reached 0.46 g PHA/g VFA. High throughput sequencing of the bacterial 16S rRNA gene confirmed that Proteobacteria and Bacteroidetes spp. increased during the enrichment and accumulation phases from 37.4% to 77.6% and from 2.49% to 17.66%, respectively. In the production of PHAs from waste streams, the presence of salts and compounds that inhibit biopolymer productivity should be taken into account. Palmeiro-Sánchez et al. [87] showed that the concentration of sodium chloride has an effect on biopolymer synthesis and accumulation. A mixed microbial culture enriched on a mixture of VFAs containing sodium chloride produced PHAs less efficiently than a culture without sodium chloride (53% of CDW).

5. Value Chain for Deriving Polyhydroxyalkanoates from VFAs

Among many different biodegradable polymers, PHAs deserve special attention due to their properties, which are similar to those of conventional plastics, as well as the fact that they are completely biodegradable to water and carbon dioxide in different environmental conditions [88]. Many efforts have been made in the past decades to increase PHA performance on both the laboratory and pilot levels. The main challenge in the commercialization of PHAs is the high production cost, which results from the low efficiency of the microbial processes.
PHAs derived from microbial processes are much more expensive than those produced using petrochemical processes. The cost of producing disposable products with P(3HB) is higher (7–10 EUR/kg) compared to production with synthetic polymers [89]. The final production costs of PHAs depend mainly on the price of the substrates used as carbon sources for microbial growth. Ensuring that the optimal carbon source is present in the microbial growth medium usually accounts for about 50% of the total cost of the PHA production process, which is why low-cost waste materials that can be effectively used to accumulate PHAs are constantly sought [90]. The conversion of waste materials to PHAs seems to be a solution to make the production of these biopolymers feasible (Figure 2) [91].
Many reports show that VFAs could be good carbon sources for PHA synthesis. However, most studies on PHA synthesis are conducted using petrochemical-derived VFAs as carbon sources. In order to reduce the overall costs of PHA production to a more reasonable level, it will be necessary to design a bioprocess that maximizes VFA production, which will be beneficial for the PHA synthesis. While the generation of large amounts of VFAs is desired, it is also necessary to prevent the toxic effect of VFAs on bacterial cells [92]. Mixed-culture PHA production offers the possibility of using renewable VFAs from wastes and industrial effluents. Utilizing fermented wastes or waste sludge as useful resources for VFA production is a promising alternative for reducing PHA production costs.
Additionally, a very important factor that affects the profitable production of PHAs from VFAs is the selection of a microbial producer that will effectively synthesize the desired bioproduct. In recent years, many microorganisms with the ability to synthesize various types of PHA have been studied. The PHA productivity of a microorganism is dependent on many factors, such as the type of carbon source, the temperature, the pH and the concentration of macro and microelements. For PHA production on a large scale, microorganisms should be able to utilize wastes as carbon sources, achieve a good growth rate and produce large amounts of PHAs. However, the concentration of fatty acids may result in toxicity for bacterial cells, that, up to a point, can be overcome by the fast growth of cells [93]. To enhance PHA productivity using VFAs, efforts can be made to use genetically recombined microorganisms. Furthermore, different types of PHAs are suitable for different applications. In particular, mcl-PHAs have gained much attention in recent years. Due to their thermoplasticity and biocompatibility, they can be used for medical or pharmaceutical applications. Thus far, only one study on the biosynthesis of mcl-PHAs has focused on substrates such as VFAs [66]. After bacterial cultivation, the downstream processing of PHA plays a crucial role in the production process. The separation of PHAs from non-PHA cell mass and their purification is technically challenging, especially considering the PHAs extraction that are formed in a wastewater treatment facility. Some downstream processing strategies have recently been comprehensively discussed by Surendran et al. [94].
Many companies have tried to increase PHA productivity and to commercialize them on the market. Currently, the bacterial polymer market is small. Scientists are making every effort to optimize the production process, e.g., by using low-cost and waste materials. To successfully implement the widespread commercial production of PHAs, the culture conditions, the microbial growth conditions and the method of PHA extraction will need to be taken into account.

6. Challenges and Future Perspectives

Biopolymers have received considerable attention in recent years as consumer preferences are shifting toward the use of biodegradable commodities. Among the various types of bio-based polymers, PHAs seem to be the next generation of environmentally friendly materials since their global market size is expected to considerably grow. Due to their useful properties, they are one of the most investigated class of biopolymers estimated to replace some of the today’s synthetic polymers. However, the major limitation for PHAs wide industrialization is the high overall cost of their production, mainly because of the price of the carbon substrate used in the microbial cultivation process. Therefore, there is still a need to find efficient substrates to maintain economic feasibility of PHAs commercialization. VFAs are promising carbon sources for PHA production. So far, the conversion of VFAs into PHAs using pure bacterial cultures has received little attention, and the majority of studies have used MMC for this purpose. Indeed, the production of PHAs by MMCs capable of effectively accumulating these polymers can be a cost-effective alternative to their production by pure bacterial cultures, which require sterile process conditions. PHA fermentation using MMC can be continuously conducted in unsterile conditions. Despite this, cultivation with a pure culture is often preferred because it usually leads to reproducible results.
To make PHA production a reality through fermentation using VFAs, there is a need to focus on a certain area, as discussed here. Additional investigations are needed to overcome some difficulties in the use of VFAs for producing PHAs. There are a number of challenges in microbial PHA synthesis from VFAs (Figure 3).
One of the main challenges is the regulation of ammonium and phosphorus in the VFA-rich fermented waste. It is known that the excess of these nutrients would promote the growth of microorganisms and reduce the PHA yield. The limited nitrogen and phosphorus conditions are of major importance for the effectiveness of the PHA synthesis process [95]. Struvite precipitation was proved to be effective in the rapid removal of these components from fermented waste with a minimal loss of VFAs [96]. Furthermore, the fermented waste should be filtered, especially in the case of PHA production by pure microbial culture [97]. Moreover, one major drawback is the toxicity of VFAs that could inhibit bacteria growth rates; therefore, optimization of the fermentation process using VFAs towards PHA production is crucial to maximize the bioproduct yield [98]. It seems to be necessary to know a proper concentration of VFAs which ensures the optimal acids metabolism to support a bacterial growth to a maximum level and high PHA productivity. Moreover, it was determined that the optimum level of VFAs available to bacteria increases the undissociated VFAs concentration inside their cytoplasm. The higher concentration of VFAs the higher dissociation that influences on the cytoplasm acidity. The reduction in a proton gradient across the membrane has an impact on the rising osmotic pressure that reduces the VFAs uptake inhibiting not only cell activity but also PHAs synthesis and accumulation. VFAs in undissociated form can penetrate the bacterial cell membrane and dissociate inside the cell, which may contribute to blocking ATP synthesis and disturbing the physiological balance [99]. Therefore, some energy must be used to restore the physiological balance in the cell, which contributes to the reduction of energy used for the growth and accumulation of PHAs by microorganisms. However, if the dissociated form of VFAs is present in high concentrations in the fermentation system then can cause an increase in ionic strength and in a consequence cell lysis [39]. Furthermore, VFAs may aggravate a decrease of pH in the culture medium and in a consequence may cause the overall bioprocess failure. In addition, VFAs-rich fermented waste may also contain ethanol, which can lead to high permeability of the cell membrane as well as suppressing the metabolism [100].
It is known that the chain-length of the VFA influences on the composition, properties and application of the synthesized PHAs. The data suggested that the feeding of mixed microbial culture with acetic and butyric acids results in the production of 3HB whereas propionic and valeric acids favor the synthesis and accumulation of 3HV [95]. Due to the poor properties, P(3HB) has limited applications; therefore, the production of PHA co-polymers with better properties is a good approach to overcome the limitations of P(3HB). By the appropriate combination of substrates and supplements, it is possible to produce PHA co-polymers of desired compositions. PHA co-polymers can be achieved by supplementing the feed with volatile fatty acids or through hydrolysates of different biowastes [101,102]. Some strategies of co-utilization were described above (Table 3).
Extensive research and development are still needed to optimize the synthesis of PHAs using VFAs. Only few microbes have been explored for their potential to produce PHAs using VFAs. Isolation and identification of new microbial cultures for a higher productivity is required. The PHAs productivity using VFAs generated in the process of anaerobic digestion of various types of waste is reported to be still too low. The major bottleneck is a downstream processing. There is a need to focus the attention in the area to recover VFAs with a higher productivity and purity. VFAs could also hamper the growth and PHAs synthesis by bacteria. Microbe engineering to tolerate VFAs as feedstocks may be an appropriate approach. Moreover, the great efforts should be made to separate VFAs from a fermentation broth using the cost-efficient method to ensure that the process of PHAs production will be economically feasible.
Advances in bioinformatics and metabolic engineering, along with expanding knowledge of microbial genomes may open many opportunities for the introduction of new metabolic pathways and modification of these pathways in pure bacterial cultures. A better understanding of genetic and metabolic regulation could lead to optimization of PHA production processes and the efficient utilization of VFAs as a source of carbon. In addition, the use of genetically modified microorganisms should be investigated as a potential method of improving PHAs production in the bioprocesses using VFAs. From a practical point of view, it is essential to construct a bacterial platform that will provide a consistent PHA molecular structure, thus ensuring stable material properties, which are essential for further applications of these polymers.

Author Contributions

Conceptualization, K.S. and J.M.-C.; writing—original draft preparation, K.S., P.O.-P., S.C., J.M.-C.; writing—review and editing, K.S., J.M.-C.; supervision, J.M.-C.; funding acquisition, J.M.-C., P.O.-P. All authors have read and agreed to the published version of the manuscript.

Funding

Karolina Szacherska is the recipient of a scholarship from the Interdisciplinary Doctoral Studies in Bioeconomy Programme (POWR.03.02.00-00-I034/16-00), which is funded by the European Social Fund. PO-P work was financed from basic funds of the Poznan University of Technology (504101/0713/SBAD/0939).

Institutional Review Board Statement

Not applicable.

Informed Consent Statement

Not applicable.

Data Availability Statement

Not applicable.

Conflicts of Interest

The authors declare no conflict of interest.

References

  1. Avérous, L. Biodegradable Multiphase Systems Based on Plasticized Starch: A Review. J. Macromol. Sci. Part C 2004, 44, 231–274. [Google Scholar] [CrossRef]
  2. Mármol, G.; Gauss, C.; Fangueiro, R. Potential of Cellulose Microfibers for PHA and PLA Biopolymers Reinforcement. Molecules 2020, 25, 4653. [Google Scholar] [CrossRef] [PubMed]
  3. Braunegg, G.; Lefebvre, G.; Genser, K.F. Polyhydroxyalkanoates, biopolyesters from renewable resources: Physiological and engineering aspects. J. Biotechnol. 1998, 65, 127–161. [Google Scholar] [CrossRef]
  4. Tsang, Y.F.; Kumar, V.; Samadar, P.; Yang, Y.; Lee, J.; Ok, Y.S.; Song, H.; Kim, K.; Kwon, E.E.; Jeon, Y.J. Production of bioplastic through food waste valorization. Environ. Int. 2019, 127, 625–644. [Google Scholar] [CrossRef]
  5. Ranganathan, S.; Dutta, S.; Moses, J.; Anandharamakrishnan, C. Utilization of food waste streams for the production of biopolymers. Heliyon 2020, 6, e04891. [Google Scholar] [CrossRef] [PubMed]
  6. Salehizadeh, H.; Van Loosdrecht, M. Production of polyhydroxyalkanoates by mixed culture: Recent trends and biotechnological importance. Biotechnol. Adv. 2004, 22, 261–279. [Google Scholar] [CrossRef]
  7. Philip, S.; Keshavarz, T.; Roy, I. Polyhydroxyalkanoates: Biodegradable polymers with a range of applications. J. Chem. Technol. Biotechnol. 2007, 82, 233–247. [Google Scholar] [CrossRef]
  8. Koller, M. Poly (hydroxyalkanoates) for Food Packaging: Application and Attempts towards Implementation. Appl. Food Bio-technol. 2014, 1, 3–15. [Google Scholar] [CrossRef]
  9. Siracusa, V.; Rocculi, P.; Romani, S.; Rosa, M.D. Biodegradable polymers for food packaging: A review. Trends Food Sci. Technol. 2008, 19, 634–643. [Google Scholar] [CrossRef]
  10. Chen, G.-Q.; Chen, X.-Y.; Wu, F.-Q.; Chen, J.-C. Polyhydroxyalkanoates (PHA) toward cost competitiveness and functionality. Adv. Ind. Eng. Polym. Res. 2020, 3, 1–7. [Google Scholar] [CrossRef]
  11. Singh, A.K.; Mallick, N. Enhanced production of SCL-LCL-PHA co-polymer by sludge-isolated Pseudomonas aeruginosa MTCC 7925. Lett. Appl. Microbiol. 2008, 46, 350–357. [Google Scholar] [CrossRef] [PubMed]
  12. Motakatla, V.R.; Mohan, S.V. Influence of aerobic and anoxic microenvironments on polyhydroxyalkanoates (PHA) production from food waste and acidogenic effluents using aerobic consortia. Bioresour. Technol. 2012, 103, 313–321. [Google Scholar] [CrossRef]
  13. Chandel, A.K.; Da Silva, S.S.; Carvalho, W.; Singh, O.V. Sugarcane bagasse and leaves: Foreseeable biomass of biofuel and bio-products. J. Chem. Technol. Biotechnol. 2011, 87, 11–20. [Google Scholar] [CrossRef]
  14. Albuquerque, M.; Martino, V.; Pollet, E.; Avérous, L.; Reis, M.A. Mixed culture polyhydroxyalkanoate (PHA) production from volatile fatty acid (VFA)-rich streams: Effect of substrate composition and feeding regime on PHA productivity, composition and properties. J. Biotechnol. 2011, 151, 66–76. [Google Scholar] [CrossRef] [PubMed]
  15. Mohan, S.V.; Motakatla, V.R.; Subhash, G.V.; Sarma, P. Fermentative effluents from hydrogen producing bioreactor as substrate for poly(β-OH) butyrate production with simultaneous treatment: An integrated approach. Bioresour. Technol. 2010, 101, 9382–9386. [Google Scholar] [CrossRef]
  16. Mohanakrishna, G.; Mohan, S.V.; Sarma, P. Utilizing acid-rich effluents of fermentative hydrogen production process as substrate for harnessing bioelectricity: An integrative approach. Int. J. Hydrogen Energy 2010, 35, 3440–3449. [Google Scholar] [CrossRef]
  17. Mohan, S.V. Harnessing of biohydrogen from wastewater treatment using mixed fermentative consortia: Process evaluation towards optimization. Int. J. Hydrogen Energy 2009, 34, 7460–7474. [Google Scholar] [CrossRef]
  18. López, J.C.; Arnáiz, E.; Merchán, L.; Lebrero, R.; Muñoz, R. Biogas-based polyhydroxyalkanoates production by Methylocystis hirsuta: A step further in anaerobic digestion biorefineries. Chem. Eng. J. 2018, 333, 529–536. [Google Scholar] [CrossRef] [Green Version]
  19. Pfaltzgraff, L.A.; De Bruyn, M.; Cooper, E.C.; Budarin, V.; Clark, J.H. Food waste biomass: A resource for high-value chemicals. Green Chem. 2013, 15, 307–314. [Google Scholar] [CrossRef]
  20. Valentino, F.; Lorini, L.; Pavan, P.; Bolzonella, D.; Majone, M. Organic Fraction of Municipal Solid Waste Conversion into Polyhydroxyalkanoates (PHA) in a Pilot Scale Anaerobic/Aerobic Process. Chem. Eng. Trans. 2019, 74. [Google Scholar] [CrossRef]
  21. Cheah, Y.-K.; Vidal-Antich, C.; Dosta, J.; Mata-Álvarez, J. Volatile fatty acid production from mesophilic acidogenic fermentation of organic fraction of municipal solid waste and food waste under acidic and alkaline pH. Environ. Sci. Pollut. Res. 2019, 26, 35509–35522. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  22. Zhou, M.; Yan, B.; Wong, J.; Zhang, Y. Enhanced volatile fatty acids production from anaerobic fermentation of food waste: A mini-review focusing on acidogenic metabolic pathways. Bioresour. Technol. 2018, 248, 68–78. [Google Scholar] [CrossRef] [PubMed]
  23. Raposo, F.; Borja, R.; Cacho, J.; Mumme, J.; Orupõld, K.; Esteves, S.; Noguerol-Arias, J.; Picard, S.; Nielfa, A.; Scherer, P.; et al. First international comparative study of volatile fatty acids in aqueous samples by chromatographic techniques: Evaluating sources of error. TrAC Trends Anal. Chem. 2013, 51, 127–143. [Google Scholar] [CrossRef]
  24. Ruan, W.; Chen, J.; Lun, S. Production of biodegradable polymer by A. eutrophus using volatile fatty acids from acidified wastewater. Process. Biochem. 2003, 39, 295–299. [Google Scholar] [CrossRef]
  25. Raganati, F.; Procentese, A.; Olivieri, G.; Russo, M.E.; Salatino, P.; Marzocchella, A. MFA of Clostridium acetobutylicum pathway: The role of glucose and xylose on the acid formation/uptake. Chem. Eng. Trans. 2014, 38, 337–342. [Google Scholar] [CrossRef]
  26. Domingos, J.M.B.; Martinez, G.A.; Scoma, A.; Fraraccio, S.; Kerckhof, F.-M.; Boon, N.; Reis, M.A.; Fava, F.; Bertin, L. Effect of Operational Parameters in the Continuous Anaerobic Fermentation of Cheese Whey on Titers, Yields, Productivities, and Microbial Community Structures. ACS Sustain. Chem. Eng. 2017, 5, 1400–1407. [Google Scholar] [CrossRef]
  27. Zheng, X.; Chen, Y.; Liu, C. Waste Activated Sludge Alkaline Fermentation Liquid as Carbon Source for Biological Nutrients Removal in Anaerobic Followed by Alternating Aerobic-Anoxic Sequencing Batch Reactors. Chin. J. Chem. Eng. 2010, 18, 478–485. [Google Scholar] [CrossRef]
  28. Dahiya, S.; Sarkar, O.; Swamy, Y.; Mohan, S.V. Acidogenic fermentation of food waste for volatile fatty acid production with co-generation of biohydrogen. Bioresour. Technol. 2015, 182, 103–113. [Google Scholar] [CrossRef]
  29. Liu, H.; Han, P.; Liu, H.; Zhou, G.; Fu, B.; Zheng, Z. Full-scale production of VFAs from sewage sludge by anaerobic alkaline fermentation to improve biological nutrients removal in domestic wastewater. Bioresour. Technol. 2018, 260, 105–114. [Google Scholar] [CrossRef]
  30. Fu, Z.; Holtzapple, M.T. Consolidated bioprocessing of sugarcane bagasse and chicken manure to ammonium carboxylates by a mixed culture of marine microorganisms. Bioresour. Technol. 2010, 101, 2825–2836. [Google Scholar] [CrossRef]
  31. Zhou, A.; Guo, Z.; Yang, C.; Kong, F.; Liu, W.; Wang, A. Volatile fatty acids productivity by anaerobic co-digesting waste activated sludge and corn straw: Effect of feedstock proportion. J. Biotechnol. 2013, 168, 234–239. [Google Scholar] [CrossRef] [PubMed]
  32. Chalima, A.; Oliver, L.; De Castro, L.F.; Karnaouri, A.; Dietrich, T.; Topakas, E. Utilization of Volatile Fatty Acids from Microalgae for the Production of High Added Value Compounds. Fermentation 2017, 3, 54. [Google Scholar] [CrossRef] [Green Version]
  33. Feng, L.; Chen, Y.; Zheng, X. Enhancement of Waste Activated Sludge Protein Conversion and Volatile Fatty Acids Accumulation during Waste Activated Sludge Anaerobic Fermentation by Carbohydrate Substrate Addition: The Effect of pH. Environ. Sci. Technol. 2009, 43, 4373–4380. [Google Scholar] [CrossRef] [PubMed]
  34. Mohan, S.V.; Butti, S.K.; Amulya, K.; Dahiya, S.; Modestra, J.A. Waste Biorefinery: A New Paradigm for a Sustainable Bioelectro Economy. Trends Biotechnol. 2016, 34, 852–855. [Google Scholar] [CrossRef] [PubMed]
  35. Arslan, D.; Steinbusch, K.J.J.; Diels, L.; Hamelers, H.V.M.; Strik, D.P.B.T.B.; Buisman, C.J.N.; De Wever, H. Selective short-chain carboxylates production: A review of control mechanisms to direct mixed culture fermentations. Crit. Rev. Environ. Sci. Technol. 2016, 46, 592–634. [Google Scholar] [CrossRef]
  36. Bermúdez-Penabad, N.; Kennes, C.; Veiga, M.C. Anaerobic digestion of tuna waste for the production of volatile fatty acids. Waste Manag. 2017, 68, 96–102. [Google Scholar] [CrossRef]
  37. Boer, J.D.; Łukaszewska, A.; Kluczkiewicz, W.; Lewandowska, D.; King, K.; Reijonen, T.; Kuhmonen, T.; Suhonen, A.; Jääskeläinen, A.; Heitto, A.; et al. Volatile fatty acids as an added value from biowaste. Waste Manag. 2016, 58, 62–69. [Google Scholar] [CrossRef]
  38. Moretto, G.; Valentino, F.; Bolzonella, D.; Majone, M.; Bolzonella, D. Optimization of urban waste fermentation for volatile fatty acids production. Waste Manag. 2019, 92, 21–29. [Google Scholar] [CrossRef]
  39. Al Battashi, H.; Al-Kindi, S.; Gupta, V.K.; Sivakumar, N. Polyhydroxyalkanoate (PHA) Production Using Volatile Fatty Acids Derived from the Anaerobic Digestion of Waste Paper. J. Polym. Environ. 2021, 29, 250–259. [Google Scholar] [CrossRef]
  40. Nayak, J.; Pal, P. Transforming Waste Cheese-Whey into Acetic Acid through a Continuous Membrane-Integrated Hybrid Process. Ind. Eng. Chem. Res. 2013, 52, 2977–2984. [Google Scholar] [CrossRef]
  41. Sim, J.H.; Kamaruddin, A.H. Optimization of acetic acid production from synthesis gas by chemolithotrophic bacterium–Clostridium aceticum using statistical approach. Bioresour. Technol. 2008, 99, 2724–2735. [Google Scholar] [CrossRef] [PubMed]
  42. Ravinder, T.; Ramesh, B.; Seenayya, G.; Reddy, G. Fermentative production of acetic acid from various pure and natural cellulosic materials by Clostridium lentocellum SG6. World J. Microbiol. Biotechnol. 2000, 16, 507–512. [Google Scholar] [CrossRef]
  43. Ehsanipour, M.; Suko, A.V.; Bura, R. Fermentation of lignocellulosic sugars to acetic acid by Moorella thermoacetica. J. Ind. Microbiol. Biotechnol. 2016, 43, 807–816. [Google Scholar] [CrossRef] [PubMed]
  44. Wang, Z.; Yan, M.; Chen, X.; Li, D.; Qin, L.; Li, Z.; Yao, J.; Liang, X. Mixed culture of Saccharomyces cerevisiae and Acetobacter pasteurianus for acetic acid production. Biochem. Eng. J. 2013, 79, 41–45. [Google Scholar] [CrossRef]
  45. Coral, J.; Karp, S.G.; Vandenberghe, L.P.D.S.; Parada, J.L.; Pandey, A.; Soccol, C.R. Batch Fermentation Model of Propionic Acid Production by Propionibacterium acidipropionici in Different Carbon Sources. Appl. Biochem. Biotechnol. 2008, 151, 333–341. [Google Scholar] [CrossRef]
  46. Zhu, Y.; Li, J.; Tan, M.; Liu, L.; Jiang, L.; Sun, J.; Lee, P.; Du, G.; Chen, J. Optimization and scale-up of propionic acid production by propionic acid-tolerant Propionibacterium acidipropionici with glycerol as the carbon source. Bioresour. Technol. 2010, 101, 8902–8906. [Google Scholar] [CrossRef]
  47. Ramsay, J.; Hassan, M.-C.A.; Ramsay, B. Biological conversion of hemicellulose to propionic acid. Enzym. Microb. Technol. 1998, 22, 292–295. [Google Scholar] [CrossRef]
  48. Gupta, A.; Srivastava, A.K. Continuous propionic acid production from cheese whey usingin situ spin filter. Biotechnol. Bioprocess Eng. 2001, 6, 1–5. [Google Scholar] [CrossRef]
  49. Feng, X.-H.; Chen, F.; Xu, H.; Wu, B.; Yao, J.; Ying, H.; Ouyang, P.-K. Propionic acid fermentation by Propionibacterium freudenreichii CCTCC M207015 in a multi-point fibrous-bed bioreactor. Bioprocess Biosyst. Eng. 2010, 33, 1077–1085. [Google Scholar] [CrossRef]
  50. Himmi, E.H.; Bories, A.; Boussaid, A.; Hassani, L. Propionic acid fermentation of glycerol and glucose by Propionibacterium acidipropionici and Propionibacterium freudenreichii ssp. shermanii. Appl. Microbiol. Biotechnol. 2000, 53, 435–440. [Google Scholar] [CrossRef]
  51. Zigová, J.; Šturdík, E.; Vandák, D. Schlosser, Štefan Butyric acid production by Clostridium butyricum with integrated extraction and pertraction. Process. Biochem. 1999, 34, 835–843. [Google Scholar] [CrossRef]
  52. He, G.; Kong, Q.; Chen, Q.-H.; Ruan, H. Batch and fed-batch production of butyric acid byClostridium butyricumZJUCB. J. Zhejiang Univ. A 2005, 6, 1076–1080. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  53. Canganella, F.; Wiegel, J. Continuous cultivation of Clostridium thermobutyricum in a rotary fermentor system. J. Ind. Microbiol. Biotechnol. 2000, 24, 7–13. [Google Scholar] [CrossRef]
  54. Jiang, L.; Wang, J.; Liang, S.; Wang, X.; Cen, P.; Xu, Z. Butyric acid fermentation in a fibrous bed bioreactor with immobilized Clostridium tyrobutyricum from cane molasses. Bioresour. Technol. 2009, 100, 3403–3409. [Google Scholar] [CrossRef] [PubMed]
  55. Wei, D.; Liu, X.; Yang, S.-T. Butyric acid production from sugarcane bagasse hydrolysate by Clostridium tyrobutyricum immobilized in a fibrous-bed bioreactor. Bioresour. Technol. 2013, 129, 553–560. [Google Scholar] [CrossRef]
  56. Raza, Z.A.; Abid, S.; Banat, I.M. Polyhydroxyalkanoates: Characteristics, production, recent developments and applications. Int. Biodeterior. Biodegrad. 2018, 126, 45–56. [Google Scholar] [CrossRef]
  57. Chakraborty, P.; Gibbons, W.; Muthukumarappan, K. Conversion of volatile fatty acids into polyhydroxyalkanoate byRalstonia eutropha. J. Appl. Microbiol. 2009, 106, 1996–2005. [Google Scholar] [CrossRef]
  58. Reddy, S.V.; Thirumala, M.; Mahmood, S.K. Production of PHB and P (3HB-co-3HV) biopolymers by Bacillus megaterium strain OU303A isolated from municipal sewage sludge. World J. Microbiol. Biotechnol. 2008, 25, 391–397. [Google Scholar] [CrossRef]
  59. Munir, S.; Jamil, N. Polyhydroxyalkanoates (PHA) production in bacterial co-culture using glucose and volatile fatty acids as carbon source. J. Basic Microbiol. 2018, 58, 247–254. [Google Scholar] [CrossRef]
  60. Ferre-Guell, A.; Winterburn, J. Increased production of polyhydroxyalkanoates with controllable composition and consistent material properties by fed-batch fermentation. Biochem. Eng. J. 2019, 141, 35–42. [Google Scholar] [CrossRef]
  61. Yun, J.H.; Sawant, S.S.; Kim, B.S. Production of polyhydroxyalkanoates by Ralstonia eutropha from volatile fatty acids. Korean J. Chem. Eng. 2013, 30, 2223–2227. [Google Scholar] [CrossRef]
  62. Martinez, G.A.; Bertin, L.; Scoma, A.; Rebecchi, S.; Braunegg, G.; Fava, F. Production of polyhydroxyalkanoates from dephenolised and fermented olive mill wastewaters by employing a pure culture of Cupriavidus necator. Biochem. Eng. J. 2015, 97, 92–100. [Google Scholar] [CrossRef]
  63. Du, G.; Si, Y.; Yu, J. Inhibitory effect of medium-chain-length fatty acids on synthesis of polyhydroxyalkanoates from volatile fatty acids by Ralstonia eutropha. Biotechnol. Lett. 2001, 23, 1613–1617. [Google Scholar] [CrossRef]
  64. Tajima, K.; Igari, T.; Nishimura, D.; Nakamura, M.; Satoh, Y.; Munekata, M. Isolation and characterization ofBacillus sp. INT005 accumulating polyhydroxyalkanoate (PHA) from gas field soil. J. Biosci. Bioeng. 2003, 95, 77–81. [Google Scholar] [CrossRef]
  65. Haywood, G.W.; Anderson, A.J.; Williams, D.R.; Dawes, E.A.; Ewing, D.F. Accumulation of a poly(hydroxyalkanoate) copolymer containing primarily 3-hydroxyvalerate from simple carbohydrate substrates by Rhodococcus sp. NCIMB 40126. Int. J. Biol. Macromol. 1991, 13, 83–88. [Google Scholar] [CrossRef]
  66. Cerrone, F.; Choudhari, S.K.; Davis, R.; Cysneiros, D.; O’Flaherty, V.; Duane, G.; Casey, E.; Guzik, M.; Kenny, S.T.; Babu, R.P.; et al. Medium chain length polyhydroxyalkanoate (mcl-PHA) production from volatile fatty acids derived from the anaerobic digestion of grass. Appl. Microbiol. Biotechnol. 2013, 98, 611–620. [Google Scholar] [CrossRef]
  67. Sudesh, K.; Abe, H.; Doi, Y. Synthesis, structure and properties of polyhydroxyalkanoates: Biological polyesters. Prog. Polym. Sci. 2000, 25, 1503–1555. [Google Scholar] [CrossRef]
  68. Arcos-Hernández, M.V.; Laycock, B.; Donose, B.C.; Pratt, S.; Halley, P.; Al-Luaibi, S.; Werker, A.; Lant, P.A. Physicochemical and mechanical properties of mixed culture polyhydroxyalkanoate (PHBV). Eur. Polym. J. 2013, 49, 904–913. [Google Scholar] [CrossRef]
  69. Kumar, P.; Ray, S.; Kalia, V.C. Production of co-polymers of polyhydroxyalkanoates by regulating the hydrolysis of biowastes. Bioresour. Technol. 2016, 200, 413–419. [Google Scholar] [CrossRef]
  70. Jeon, J.-M.; Kim, H.-J.; Bhatia, S.K.; Sung, C.; Seo, H.-M.; Kim, J.-H.; Park, H.-Y.; Lee, D.; Brigham, C.J.; Yang, Y.-H. Application of acetyl-CoA acetyltransferase (AtoAD) in Escherichia coli to increase 3-hydroxyvalerate fraction in poly(3-hydroxybutyrate-co-3-hydroxyvalerate). Bioprocess Biosyst. Eng. 2017, 40, 781–789. [Google Scholar] [CrossRef]
  71. Koller, M.; Hesse, P.; Bona, R.; Kutschera, C.; Atlić, A.; Braunegg, G. Potential of Various Archae- and Eubacterial Strains as Industrial Polyhydroxyalkanoate Producers from Whey. Macromol. Biosci. 2007, 7, 218–226. [Google Scholar] [CrossRef] [PubMed]
  72. Reis, M.A.M.; Serafim, L.S.; Lemos, P.C.; Reis, M.A.; Aguiar, F.R.; Van Loosdrecht, M.C.M. Production of polyhydroxyalkanoates by mixed microbial cultures. Bioprocess Biosyst. Eng. 2003, 25, 377–385. [Google Scholar] [CrossRef] [PubMed]
  73. Serafim, L.S.; Lemos, P.C.; Oliveira, R.; Reis, M.A. Optimization of polyhydroxybutyrate production by mixed cultures submitted to aerobic dynamic feeding conditions. Biotechnol. Bioeng. 2004, 87, 145–160. [Google Scholar] [CrossRef]
  74. Beun, J.; Dircks, K.; Van Loosdrecht, M.; Heijnen, J. Poly-β-hydroxybutyrate metabolism in dynamically fed mixed microbial cultures. Water Res. 2002, 36, 1167–1180. [Google Scholar] [CrossRef]
  75. Johnson, K.; Jiang, Y.; Kleerebezem, R.; Muyzer, G.; Van Loosdrecht, M.C.M. Enrichment of a Mixed Bacterial Culture with a High Polyhydroxyalkanoate Storage Capacity. Biomacromolecules 2009, 10, 670–676. [Google Scholar] [CrossRef]
  76. Fradinho, J.; Oehmen, A.; Reis, M.A. Photosynthetic mixed culture polyhydroxyalkanoate (PHA) production from individual and mixed volatile fatty acids (VFAs): Substrate preferences and co-substrate uptake. J. Biotechnol. 2014, 185, 19–27. [Google Scholar] [CrossRef]
  77. Chua, A.S.M.; Takabatake, H.; Satoh, H.; Mino, T. Production of polyhydroxyalkanoates (PHA) by activated sludge treating municipal wastewater: Effect of pH, sludge retention time (SRT), and acetate concentration in influent. Water Res. 2003, 37, 3602–3611. [Google Scholar] [CrossRef]
  78. Bengtsson, S.; Werker, A.; Christensson, M.; Welander, T. Production of polyhydroxyalkanoates by activated sludge treating a paper mill wastewater. Bioresour. Technol. 2008, 99, 509–516. [Google Scholar] [CrossRef] [PubMed]
  79. Chen, H.; Meng, H.; Nie, Z.; Zhang, M. Polyhydroxyalkanoate production from fermented volatile fatty acids: Effect of pH and feeding regimes. Bioresour. Technol. 2013, 128, 533–538. [Google Scholar] [CrossRef] [PubMed]
  80. Farghaly, A.; Enitan, A.M.; Kumari, S.; Bux, F.; Tawfik, A. Polyhydroxyalkanoates production from fermented paperboard mill wastewater using acetate-enriched bacteria. Clean Technol. Environ. Policy 2016, 19, 935–947. [Google Scholar] [CrossRef]
  81. Liao, Q.; Gao, M.; Ran, Y.; Gao, M.; She, Z.; Zhao, Y.; Liu, Y. Optimization of polyhydroxyalkanoates (PHA) synthesis with heat pretreated waste sludge. Waste Manag. 2018, 82, 15–25. [Google Scholar] [CrossRef] [PubMed]
  82. Burniol-Figols, A.; Varrone, C.; Le, S.B.; Daugaard, A.E.; Skiadas, I.V.; Gavala, H.N. Combined polyhydroxyalkanoates (PHA) and 1,3-propanediol production from crude glycerol: Selective conversion of volatile fatty acids into PHA by mixed microbial consortia. Water Res. 2018, 136, 180–191. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  83. Li, D.; Yin, F.; Ma, X. Towards biodegradable polyhydroxyalkanoate production from wood waste: Using volatile fatty acids as conversion medium. Bioresour. Technol. 2020, 299, 122629. [Google Scholar] [CrossRef] [PubMed]
  84. Fradinho, J.; Oehmen, A.; Reis, M. Improving polyhydroxyalkanoates production in phototrophic mixed cultures by optimizing accumulator reactor operating conditions. Int. J. Biol. Macromol. 2019, 126, 1085–1092. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  85. Lemos, P.C.; Serafim, L.S.; Reis, M.A. Synthesis of polyhydroxyalkanoates from different short-chain fatty acids by mixed cultures submitted to aerobic dynamic feeding. J. Biotechnol. 2006, 122, 226–238. [Google Scholar] [CrossRef]
  86. Ciesielski, S.; Przybylek, G. Volatile fatty acids influence on the structure of microbial communities producing PHAs. Braz. J. Microbiol. 2014, 45, 395–402. [Google Scholar] [CrossRef] [Green Version]
  87. Palmeiro-Sánchez, T.; Fra-Vázquez, A.; Rey-Martínez, N.; Campos, J.; Mosquera-Corral, A. Transient concentrations of NaCl affect the PHA accumulation in mixed microbial culture. J. Hazard. Mater. 2016, 306, 332–339. [Google Scholar] [CrossRef] [PubMed]
  88. Godbole, S. Methods for identification, quantification and characterization of polyhydroxyalkanoates. Int. J. Bioassays 2016, 5, 4977. [Google Scholar] [CrossRef]
  89. Bhatt, R.; Patel, K.; Trivedi, U. Chapter 10. Biodegradation of Poly (3-Hydroxyalkanoates); Royal Society of Chemistry (RSC): London, UK, 2011; pp. 311–331. [Google Scholar]
  90. Lee, S.H.; Kim, J.H.; Mishra, D.; Ni, Y.-Y.; Rhee, Y.H. Production of medium-chain-length polyhydroxyalkanoates by activated sludge enriched under periodic feeding with nonanoic acid. Bioresour. Technol. 2011, 102, 6159–6166. [Google Scholar] [CrossRef] [PubMed]
  91. Sun, Z.; Ramsay, J.A.; Guay, M.; Ramsay, B.A. Fermentation process development for the production of medium-chain-length poly-3-hyroxyalkanoates. Appl. Microbiol. Biotechnol. 2007, 75, 475–485. [Google Scholar] [CrossRef]
  92. Bhattacharyya, J.; Kumar, S.; Devotta, S. Studies on acidification in two-phase biomethanation process of municipal solid waste. Waste Manag. 2008, 28, 164–169. [Google Scholar] [CrossRef] [PubMed]
  93. Kourmentza, C.; Plácido, J.; Venetsaneas, N.; Burniol-Figols, A.; Varrone, C.; Gavala, H.N.; Reis, M.A. Recent Advances and Challenges towards Sustainable Polyhydroxyalkanoate (PHA) Production. Bioengineering 2017, 4, 55. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  94. Surendran, A.; Lakshmanan, M.; Chee, J.Y.; Sulaiman, A.M.; Van Thuoc, D.; Sudesh, K. Can Polyhydroxyalkanoates Be Produced Efficiently From Waste Plant and Animal Oils? Front. Bioeng. Biotechnol. 2020, 8, 169. [Google Scholar] [CrossRef] [PubMed]
  95. Lee, W.S.; Chua, A.S.M.; Yeoh, H.K.; Ngoh, G.C. A review of the production and applications of waste-derived volatile fatty acids. Chem. Eng. J. 2014, 235, 83–99. [Google Scholar] [CrossRef]
  96. Mengmeng, C.; Hong, C.; Qingliang, Z.; Shirley, S.N.; Jie, R. Optimal production of polyhydroxyalkanoates (PHA) in activated sludge fed by volatile fatty acids (VFAs) generated from alkaline excess sludge fermentation. Bioresour. Technol. 2009, 100, 1399–1405. [Google Scholar] [CrossRef] [PubMed]
  97. Albuquerque, M.; Eiroa, M.; Torres, C.; Nunes, B.; Reis, M.A. Strategies for the development of a side stream process for polyhydroxyalkanoate (PHA) production from sugar cane molasses. J. Biotechnol. 2007, 130, 411–421. [Google Scholar] [CrossRef]
  98. Ji, J.-Y.; Xing, Y.-J.; Ma, Z.-T.; Zhang, M.; Zheng, P. Acute toxicity of pharmaceutical wastewaters containing antibiotics to anaerobic digestion treatment. Chemosphere 2013, 91, 1094–1098. [Google Scholar] [CrossRef]
  99. Sun, C.Q.; O’Connor, C.J.; Turner, S.J.; Lewis, G.D.; Stanley, R.A.; Roberton, A.M. The effect of pH on the inhibition of bacterial growth by physiological concentrations of butyric acid: Implications for neonates fed on suckled milk. Chem. Interactions 1998, 113, 117–131. [Google Scholar] [CrossRef]
  100. Zeb, B.S.; Mahmood, Q.; Ping, Z.; Lin, Q.; Lu, H.; Tingting, C.; Abbas, G. Assessment of toxicity of volatile fatty acids to Pho-tobacterium phosphoreum. Microbiology 2014, 83, 510–515. [Google Scholar] [CrossRef]
  101. Ray, S.; Kalia, V.C. Microbial Cometabolism and Polyhydroxyalkanoate Co-polymers. Indian J. Microbiol. 2016, 57, 39–47. [Google Scholar] [CrossRef]
  102. Ray, S.; Sharma, R.; Kalia, V.C. Co-utilization of Crude Glycerol and Biowastes for Producing Polyhydroxyalkanoates. Indian J. Microbiol. 2017, 58, 33–38. [Google Scholar] [CrossRef]
Polymers 13 00321 g001 550
Figure 1. Scheme of metabolic pathways for volatile fatty acids production and polyhydroxyalkanoates synthesis. ack—acetate kinase, acul—acrylyl-CoA reductase, adh—alcohol dehydrogenase, ald—aldehyde dehydrogenase, alsS—acetolactate synthase, aor—aldehyde oxidoreductase, bcd—butyryl-CoA dehydrogenase, bk—butyrate kinase, crt—crotonase, hbd—hydroxybutyryl-CoA dehydrogenase, ilvc— keto-acid reductoisomerase, ilvD—dihydroxy acid dehydratase, kivD—2-keto acid decarboxylase, lcdA—lactoyl-CoA dehydratase, ldh—lactate dehydrogenase, leuA—2-isopropylmalate synthase, leuB—isopropylmalate dehydrogenase, leuCD—isopropylmalate isomerase complex, pct—propionyl-CoA transferase, pta—phosphotransacetylase, ptb—phosphotransbutyrylase, thl—thiolase.
Figure 1. Scheme of metabolic pathways for volatile fatty acids production and polyhydroxyalkanoates synthesis. ack—acetate kinase, acul—acrylyl-CoA reductase, adh—alcohol dehydrogenase, ald—aldehyde dehydrogenase, alsS—acetolactate synthase, aor—aldehyde oxidoreductase, bcd—butyryl-CoA dehydrogenase, bk—butyrate kinase, crt—crotonase, hbd—hydroxybutyryl-CoA dehydrogenase, ilvc— keto-acid reductoisomerase, ilvD—dihydroxy acid dehydratase, kivD—2-keto acid decarboxylase, lcdA—lactoyl-CoA dehydratase, ldh—lactate dehydrogenase, leuA—2-isopropylmalate synthase, leuB—isopropylmalate dehydrogenase, leuCD—isopropylmalate isomerase complex, pct—propionyl-CoA transferase, pta—phosphotransacetylase, ptb—phosphotransbutyrylase, thl—thiolase.
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Figure 2. PHAs process value chain using volatile fatty acids.
Figure 2. PHAs process value chain using volatile fatty acids.
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Figure 3. Challenges in producing polyhydroxyalkanoate biopolymers using VFAs.
Figure 3. Challenges in producing polyhydroxyalkanoate biopolymers using VFAs.
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Table
Table 1. Properties of volatile fatty acids [22,23].
Table 1. Properties of volatile fatty acids [22,23].
Volatile Fatty AcidBoiling Point (°C)Solubility (g/dm3)CODequivalent (g COD/g)Vapor Pressure (mm Hg)Smell
Acetic acid117Complete1.06620.9Sharp smell of vinegar
Propionic acid141Complete1.5123.3Sharp, rancid, acrid
Butyric acid164Complete1.8161.65Rancid butter, sweat
Isovaleric acid177202.0371Rancid fat, blue cheese
Valeric acid186402.0371Sweat, valerian
Caproic acid206112.2040.2Sharp, sour
Table
Table 3. Production of PHAs by pure bacterial cultures using volatile fatty acids.
Table 3. Production of PHAs by pure bacterial cultures using volatile fatty acids.
BacteriaType of PHACarbon SourceBiomass (g/L)PHA Content (%)PHA Productivity (g/L/h)References
Ralstonia eutropha ATCC 17699P(3HB)acetic acid5.430.80.013[57]
propionic acid14.029.30.036
butyric acid14.531.90.037
Bacillus megaterium OU303AP(3HB)propionic acid + glucosend62.4nd[58]
propionic acid + glycerolnd57.2nd
Pseudomonas sp. ST2P(3HB-co-3HV)propionic acid + glucosend34.0nd[59]
Bacillus sp. CS8propionic acid + glucosend24.0nd
Pseudomonas sp. ST2 + Bacillus sp. CS8acetic acid+ propionic acid + glucosend35.0nd
Haloferax mediterraneiP(3HB-co-3HV)butyric acid + valeric acid + Tween 20nd58.90.010[60]
Ralstonia eutropha ATCC 17699P(3HB-co-3HV)acetic acid + propionic acid + butyric acid1.225.0nd[61]
Ralstonia eutropha KCTC 2658P(3HB-co-3HV)acetic acid + propionic acid + butyric acid1.550.0nd
Cupriavidus necatorP(3HB-co-3HV)olive mill wastewater effluent rich in acetic, propionic and butyric acid2.055.00.022[62]
Methylocystis hirsuta DSM 18500P(3HB-co-3HV)acetic acidnd2.4nd[18]
propionic acidnd1.1nd
butyric acidnd1.8nd
valeric acidnd9.0nd
P(3HB)acetic acid + biogasnd52.3nd
P(3HB-co-3HV)propionic acid + biogasnd47.9nd
P(3HB)butyric acid + biogasnd52.2nd
P(3HB-co-3HV)valeric acid + biogasnd53.8nd
Ralstonia eutropha DSM 545P(3HB-co-3HV)glucose + propionic acid52.178.30.74[63]
Bacillus sp. INT005P(3HB)butyric acid0.831.5nd[64]
P(3HB-co-3HV)valeric acid0.718.8nd
Corynebacterium hydrocarboxydansP(3HB-co-3HV)acetic acidnd21.0nd[65]
Nocardia lucidaP(3HB-co-3HV)acetic acidnd20.0nd
Rhodococcus sp.P(3HB-co-3HV)acetic acidnd29.0nd
P(3HB-co-3HV)valeric acidnd43.0nd
Pseudomonas putida KT2440mcl-PHAacetic acid~0.526.0nd[66]
propionic acid~0.529.0nd
butyric acid~0.544.0nd
valeric acid~0.519.0nd
Pseudomonas putida CA-3acetic acid~0.6~40.0nd
propionic acid~0.6~40.0nd
butyric acid0.7~40.0nd
valeric acid~0.624.0nd
Pseudomonas putida GO16acetic acid0.4~10.0nd
propionic acid0.1~10.0nd
butyric acid0.828.0nd
valeric acid0.2~10.0nd
nd—not determined.
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Szacherska, K.; Oleskowicz-Popiel, P.; Ciesielski, S.; Mozejko-Ciesielska, J. Volatile Fatty Acids as Carbon Sources for Polyhydroxyalkanoates Production. Polymers 2021, 13, 321. https://doi.org/10.3390/polym13030321

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Szacherska K, Oleskowicz-Popiel P, Ciesielski S, Mozejko-Ciesielska J. Volatile Fatty Acids as Carbon Sources for Polyhydroxyalkanoates Production. Polymers. 2021; 13(3):321. https://doi.org/10.3390/polym13030321

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Szacherska, Karolina, Piotr Oleskowicz-Popiel, Slawomir Ciesielski, and Justyna Mozejko-Ciesielska. 2021. "Volatile Fatty Acids as Carbon Sources for Polyhydroxyalkanoates Production" Polymers 13, no. 3: 321. https://doi.org/10.3390/polym13030321

APA Style

Szacherska, K., Oleskowicz-Popiel, P., Ciesielski, S., & Mozejko-Ciesielska, J. (2021). Volatile Fatty Acids as Carbon Sources for Polyhydroxyalkanoates Production. Polymers, 13(3), 321. https://doi.org/10.3390/polym13030321

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