Enzymatic Synthesis of Biobased Polyesters and Polyamides

Nowadays, “green” is a hot topic almost everywhere, from retailers to universities to industries; and achieving a green status has become a universal aim. However, polymers are commonly considered not to be “green”, being associated with massive energy consumption and severe pollution problems (for example, the “Plastic Soup”) as a public stereotype. To achieve green polymers, three elements should be entailed: (1) green raw materials, catalysts and solvents; (2) eco-friendly synthesis processes; and (3) sustainable polymers with a low carbon footprint, for example, (bio)degradable polymers or polymers which can be recycled or disposed with a gentle environmental impact. By utilizing biobased monomers in enzymatic polymerizations, many advantageous green aspects can be fulfilled. For example, biobased monomers and enzyme catalysts are renewable materials that are derived from biomass feedstocks; enzymatic polymerizations are clean and energy saving processes; and no toxic residuals contaminate the final products. Therefore, synthesis of renewable polymers via enzymatic polymerizations of biobased monomers provides an opportunity for achieving green polymers and a future sustainable polymer industry, which will eventually play an essential role for realizing and maintaining a biobased and sustainable society.

chemical structures; and it is nearly impossible to produce biobased polymers with identical structures as the petrol-based counterparts, due to the use of biomolecule mixtures. Besides, some unwanted structures or impurities might be inherited from the biomolecule mixtures, which might greatly influence the properties and applications of the final polymeric materials.
Utilization of biobased monomers with tailored structures in polymer synthesis is the most promising approach towards biobased polymers, which can result in not only sustainable alternatives to petrol-based counterparts with similar or identical structures, but also in novel green polymers that cannot be produced from petrol-based monomers [5,8,9,[14][15][16]. However, this is also the most expensive approach of all three as aforementioned.
Enzymatic polymerization is an emerging alternative approach for the production of polymeric materials, which can compete against conventional chemical synthesis and physical modification techniques [35][36][37][38][39][40][41][42][43][44]. Enzymatic polymerization also provides a great opportunity for accessing novel macromolecules that are not accessible via conventional approaches. Moreover, with mild synthetic conditions and renewable non-toxic enzyme catalysts, enzymatic polymerization is considered as an effective way to reduce the dependence of fossil resources and to address the high material consumption and pollution problems in the polymer industry.
At present, petrol-based monomers are still predominately used in enzymatic polymerizations. By combining biobased monomers and enzymatic polymerizations in polymer synthesis, not only the research field of enzymatic polymerization could be greatly accelerated but also the utilization of renewable resources will be promoted. This will provide an essential contribution for achieving sustainability for the polymer industry, which will eventually play an important role for realizing and maintaining a sustainable society.
in the market, with a global production of 2.1 million tons. Actually, nylon 6,6 is the first example of aliphatic polyamides, which was firstly produced in the laboratory by Carothers and Hill at DuPont in 1930. After that, this polyamide was prepared by DuPont as nylon 6,6 fiber on 28 February 1935, and then produced at full-scale in July 1935. Regarding nylon 6, it was firstly developed by Schlack at IG Farbenindustrie in 1938, for the purpose of reproducing the properties of nylon 6,6 without violating the patents [70,71]. At present, 66% of nylon 6 production is used as fibers, 30% is applied as engineering thermoplastics, and the rest 10% is consumed as films. For nylon 6,6, 55% of the current production is used as fibers, and the remainder is applied as engineering thermoplastics. Other nylons like nylon 4,10, nylon 6,12, nylon 10,10, nylon 11 and nylon 12 are commonly used as high performance materials [72].
Semi-aromatic polyamides consist of both aliphatic and aromatic fragments in the polymer main chain. Especially, polyphthalamides (PPAs), a type of semi-aromatic polyamides, are defined by ASTM D5336 as "polyamides in which at least 55 mol % of the carboxylic acid portion of the repeating unit in the polymer chain is comprised by a combination of terephthalic acid (TPA) and isophthalic acid (IPA)" [73]. Compared to aliphatic polyamides, semi-aromatic polyamides are much stiffer, rendering the polyamides with higher mechanical strength and better thermal resistance. In addition, semi-aromatic polyamides possess many other merits such as high heat chemical/abrasion/corrosion resistance, good dimensional stability, superior processing characteristics and direct bonding to many elastomers. Semi-aromatic polyamides can be used as thermal engineering materials and high performance materials, which have found various applications in many areas, for example, in marine, automotive industry, oil industry, electronics, machinery, domestic appliances, medical devices, personal care, and so on. Examples of semi-aromatic polyamides are PA 6,T, poly(nonamethylene terephthalamide) (PA 9,T), and poly(decamethylene terephthalamide) (PA 10,T). They are commercially produced by many companies such as DuPont (Zytel ® HTN, PA 6,T), Solvay (Amodel ® , PA 6,T), EMS-GRIVORY (Grilamid ® HT, PA 6,T), Mitsui (ARLEN ® , PA 6,T/6,6), Kuraray (Genesta ® , PA 9,T), and Evonik (VESTAMID ® HTplus, PA 6,T/X or PA 10,T/X) [72,74].
Aromatic polyamides are normally referred to wholly aromatic polyamides, or aramids in which at least 85% of the amide linkages are directly attached to two aromatic groups [73,75,76]. Due to the amide linkages and the rigid aromatic structures, the stiff rod-like aromatic polyamide chains interact with each other by strong and highly directional hydrogen bonds and π-π stackings. Therefore, aromatic polyamides possess outstanding thermal and mechanical resistance, and excellent chemically inert property, but a poor solubility and processability. Aromatic polyamides are high performance materials that are used as advantageous replacement for metals or ceramics, cut-resistant, flame resistant and high-tensile strength synthetic fibers and coatings, bullet-proof body armor, protective clothing, electrical insulation materials, sealing materials, composites, and so on. Examples of aromatic polyamides are PPPTA and poly(m-phenylene isophthalamide) (PMPI). These two aramids are the most well-known commercially available aromatic polyamides, with the trademark of Kevlar ® (DuPont) and Nomex ® (DuPont), respectively. Besides, some aromatic polyamides display liquid crystalline properties. For example, the solid-state PPPT (Kevlar ® , DuPont, Wilmington, DE, USA) is an example of main chain lyotropic liquid crystal polymers [55].
Regarding the equipment and the reaction conditions followed, the polymerization steps in polyester and polyamide synthesis are similar [57]. However, with respect to the formation of high molecular weight products, the polymerization of polyamides differs from that of polyesters to some extent. Firstly, the chemical equilibrium is favored for the amide formation but is less favored for the ester formation. Secondly, when dicarboxylic acids are used as starting materials, salts are formed in polyamide synthesis, but there is no salt formation in polyester synthesis. In this case, stoichiometric equivalence can be much more easily achieved in polyamide synthesis. Thirdly, the amide interchange reactions (transamidations) are much slower than the ester interchange reactions (transesterifications).

Biobased Monomers for Polyester and Polyamide Synthesis
Generally speaking, lactones, diacids and their ester and anhydride derivatives, diols, polyols, and hydroxyacids and their esters are good building blocks for polyester synthesis, while lactams, ω-amino acids and their esters, diacids and their derivatives, and diamines are suitable monomers for polyamide synthesis. Herein, some predominate biobased monomers for polyester and polyamide synthesis are outlined.

Biobased Lactones and Lactams
Lactones and lactams are abundant moieties in naturally occurring compounds with diversified structures and varied ring sizes. Examples of naturally occurred lactones and lactams are tetronic acid, 5,6-dihydropyran-2-one, coumarin, α-alkylidene-γ-lactones and lactams, α-alkylidene-δ-lactones and lactams, β-lactam, and so on. They are widely applied in the fine and functional perfumery and in the pharmaceutical industry. However, few studies referred to the synthesis of polyesters and polyamides from naturally occurring lactones and lactams, probably due to their complicated structures, limited availability, and high price [77].
3-Hydroxybutyrolactone (3-HBL) is a biobased platform molecules listed in "DOE TOP 10" [18]. It is a chiral compound that can be used for the synthesis of pharmaceuticals, polymers and organic solvents. However, the chemical synthesis of 3-HBL is quite difficult, with multiple steps [5,18,78]. Currently, (S)-3-HBL is commercially produced from L-malic acid via a continuous chemical synthesis process under high pressure in a fixed-bed reactor using a ruthenium-based catalyst [79,80] This process involves hazardous conditions, expensive catalysts, as well as multiple purification steps [78]. Recently, Prather et al. [78,81] developed a biosynthesis pathway for 3-HBL in recombinant E. coli (Escherichia coli) using glycolic acid or glucose as the starting material. However, the large-scale biological production of 3-HBL is still challenging, which requires further studies.
In addition, lactams can be converted from biomass feedstocks. Among them, ε-caprolactam is an important raw material for the synthesis of nylon 6. At present, ε-caprolactam is produced via a six-step chemical process using benzene and ammonia as starting materials. Recently Heeres et al. [83] reported the conversion of biobased 5-(hydroxymethyl)furfural (HMF) to ε-caprolactam via four steps (Scheme 3), two steps less than the traditional approach. In addition, Bouwman et al. [84] reported the production of ε-caprolactam from biobased levulinic acid via a four-step process. Moreover, synthesis of ε-caprolactam from sugar-derived lysine is developed [85,86]. It is also possible to produce ε-caprolactam via fermentation of sugars and the relevant industrial process is currently under development [31]. synthesis process under high pressure in a fixed-bed reactor using a ruthenium-based catalyst [79,80] This process involves hazardous conditions, expensive catalysts, as well as multiple purification steps [78]. Recently, Prather et al. [78,81] developed a biosynthesis pathway for 3-HBL in recombinant E. coli (Escherichia coli) using glycolic acid or glucose as the starting material. However, the large-scale biological production of 3-HBL is still challenging, which requires further studies. Some other lactones, such as propiolactone, γ-butyrolactone, angelilactone, γ-valerolactone, and furan-2(5H)-one, can be derived from renewable resources [18,82].
In addition, lactams can be converted from biomass feedstocks. Among them, ε-caprolactam is an important raw material for the synthesis of nylon 6. At present, ε-caprolactam is produced via a six-step chemical process using benzene and ammonia as starting materials. Recently Heeres et al. [83] reported the conversion of biobased 5-(hydroxymethyl)furfural (HMF) to ε-caprolactam via four steps (Scheme 3), two steps less than the traditional approach. In addition, Bouwman et al. [84] reported the production of ε-caprolactam from biobased levulinic acid via a four-step process. Moreover, synthesis of ε-caprolactam from sugar-derived lysine is developed [85,86]. It is also possible to produce ε-caprolactam via fermentation of sugars and the relevant industrial process is currently under development [31].

Biobased Aliphatic Diacids
Succinic acid is a naturally occurring dicarboxylic acid, which is predominantly produced commercially through petrochemical routes by catalytic hydrogenation of maleic acid or anhydride, with a global production of 30-50 kilo tons per year [87,88]. Succinic acid can be also produced by fermentation of carbohydrates or glycerol using engineered bacteria or yeast. The current bio-route for succinic acid is based on proprietary E. coli or yeast strains [88]. To lower the cost, other microorganisms and yeast have been developed, like Coryne-type bacteria, which shows a significantly higher productivity compared to E. coli. [33] Currently, four companies have built up commercial facilities for the production of biobased succinic acid: Reverdia, Succinity, Bioamber and Myriant [29].
Itaconic acid is an attractive unsaturated monomer that has already been produced industrially by sugar fermentation using Aspergillus terreus early in the 1960s [89,90]. The current production of itaconic acid is around 80 kilo tons per year, mainly in USA, China, Japan and France [91]. To reduce the cost and increase the sustainability, current studies mainly focus on strain improvement of microorganisms by mutagenesis, development of more cost-effective process methodologies, and the use of alternative cheap substrates such as cellulolytic biomass [91].
Adipic acid is one the most important commodity chemicals, which is mainly used for the production of nylon 6,6 [33,92]. The current global market for adipic acid is around 4 million tons per year [31]. At present, over 90% of adipic acid is manufactured industrially by oxidation of cyclohexanol or KA-oil (a mixture of cyclohexanol and cyclohexanone) using concentrated nitric acid Scheme 3. Synthesis of ε-caprolactam from biobased chemicals.

Biobased Aliphatic Diacids
Succinic acid is a naturally occurring dicarboxylic acid, which is predominantly produced commercially through petrochemical routes by catalytic hydrogenation of maleic acid or anhydride, with a global production of 30-50 kilo tons per year [87,88]. Succinic acid can be also produced by fermentation of carbohydrates or glycerol using engineered bacteria or yeast. The current bio-route for succinic acid is based on proprietary E. coli or yeast strains [88]. To lower the cost, other microorganisms and yeast have been developed, like Coryne-type bacteria, which shows a significantly higher productivity compared to E. coli. [33] Currently, four companies have built up commercial facilities for the production of biobased succinic acid: Reverdia, Succinity, Bioamber and Myriant [29].
Itaconic acid is an attractive unsaturated monomer that has already been produced industrially by sugar fermentation using Aspergillus terreus early in the 1960s [89,90]. The current production of itaconic acid is around 80 kilo tons per year, mainly in USA, China, Japan and France [91]. To reduce the cost and increase the sustainability, current studies mainly focus on strain improvement of microorganisms by mutagenesis, development of more cost-effective process methodologies, and the use of alternative cheap substrates such as cellulolytic biomass [91].
Adipic acid is one the most important commodity chemicals, which is mainly used for the production of nylon 6,6 [33,92]. The current global market for adipic acid is around 4 million tons per year [31]. At present, over 90% of adipic acid is manufactured industrially by oxidation of cyclohexanol or KA-oil (a mixture of cyclohexanol and cyclohexanone) using concentrated nitric acid [92][93][94][95]. In recent years, two prospective biosynthetic pathways to biobased adipic acid have been developed and are under commercialization evaluation at the moment [31,33]: (1) chemo-catalytic conversion of biologically derived precursors such as cis,cis-muconic acid or D-glucaric acid; and (2) direct biological conversion of vegetable oils and sugars using yeast.
1,4-Butanediol (1,4-BDO) is widely used as a building block for polymer synthesis, with an annual global market of over 2.5 million tons [104]. The industrial production of 1,4-BDO dominantly depends on petrol-based chemicals such as maleic anhydride, acetylene, butane, propylene and butadiene. Since late 2007, Genomatica (USA) started to develop a biological process for the synthesis of biobased 1,4-BDO from sugars using a genetically-modified strain of E. coli bacteria [99,[104][105][106]. This process has already been commercialized [31]. Alternatively, biobased 1,4-BDO can be produced by reduction of sugar-derived succinic acid and this process is under commercialization preparation stage [31].
1,4:3,6-Dianhydrohexitols (DAHs) are sugar-derived aliphatic diols with rigid and chiral structures [107]. It is of great interest to synthesize DAH-based polymers with high glass transition temperatures (T g ) and/or with special optical properties [108]. According to the chirality, DAHs have three possible stereoisomers: isosorbide, isomanide and isoidide (Scheme 4). Due to the different positions of the hydroxyl groups, the reactivity of these isomers are different, showing the following sequence: isomannide < isosorbide < isoidide [107,108]. Nowadays, only isosorbide is produced at an industrial scale using sugars as the starting materials [26,107]; and Roquette (France) is a leading producer. However, the purity and high price of the commercial isosorbide are two major concerns when used for polyester synthesis.  [92][93][94][95]. In recent years, two prospective biosynthetic pathways to biobased adipic acid have been developed and are under commercialization evaluation at the moment [31,33]: (1) chemo-catalytic conversion of biologically derived precursors such as cis,cis-muconic acid or D-glucaric acid; and (2) direct biological conversion of vegetable oils and sugars using yeast. In addition, suberic acid, sebacic acid and dodecanedioic acid are also (potentially) biobased monomers which can be converted from plant oils [31,[96][97][98].
1,4-Butanediol (1,4-BDO) is widely used as a building block for polymer synthesis, with an annual global market of over 2.5 million tons [104]. The industrial production of 1,4-BDO dominantly depends on petrol-based chemicals such as maleic anhydride, acetylene, butane, propylene and butadiene. Since late 2007, Genomatica (USA) started to develop a biological process for the synthesis of biobased 1,4-BDO from sugars using a genetically-modified strain of E. coli bacteria [99,[104][105][106]. This process has already been commercialized [31]. Alternatively, biobased 1,4-BDO can be produced by reduction of sugar-derived succinic acid and this process is under commercialization preparation stage [31]. 1,4:3,6-Dianhydrohexitols (DAHs) are sugar-derived aliphatic diols with rigid and chiral structures [107]. It is of great interest to synthesize DAH-based polymers with high glass transition temperatures (Tg) and/or with special optical properties [108]. According to the chirality, DAHs have three possible stereoisomers: isosorbide, isomanide and isoidide (Scheme 4). Due to the different positions of the hydroxyl groups, the reactivity of these isomers are different, showing the following sequence: isomannide < isosorbide < isoidide [107,108]. Nowadays, only isosorbide is produced at an industrial scale using sugars as the starting materials [26,107]; and Roquette (France) is a leading producer. However, the purity and high price of the commercial isosorbide are two major concerns when used for polyester synthesis. Other aliphatic diols such as 2,3-butanediol, 1,6-hexanediol, 1,8-octanediol and 1,10-decanediol, are (potentially) biobased monomers [5,109,110].
Moreover, glycerol and D-sorbitol are abundant and inexpensive biobased aliphatic polyols. Glycerol is obtained as a byproduct in the production of biodiesel from vegetable oils and fats [5,111], while D-sorbitol is produced industrially on large scale by reduction of glucose derived from biomass feedstocks [33].

Biobased Aliphatic Diamines
Moreover, glycerol and D-sorbitol are abundant and inexpensive biobased aliphatic polyols. Glycerol is obtained as a byproduct in the production of biodiesel from vegetable oils and fats [5,111], while D-sorbitol is produced industrially on large scale by reduction of glucose derived from biomass feedstocks [33].
Furthermore, sugars like glucose and sucrose, and sugar alcohols such as erythritol, xylitol and sorbitol, are polyols with multi hydroxyl groups. They are naturally occurring compounds which can be produced via fermentation of various sources of biomass feedstocks [112].
1,5-Pentanediamine (1,5-PDA, cadaverine) is a naturally occurring compound which is produced by hydrolysis of protein during the tissue putrefaction of animals, the same as 1,4-BDA. 1,5-PDA can be used for the production of nylon 5,6 and nylon 5,10. The industrial production of 1,5-PDA is similar to that of 1,4-BDA, using petrol-based 1,5-dichloropentane, glutarodinitrile, or glutaraldehyde as the starting material [114]. Moreover, the biosynthesis of 1,5-PDA is well established, by decarboxylation of lysine using several microorganisms [115,116]. It is also promising to produce biobased 1,5-PDA via fermentation of sugars by metabolic engineering. Currently, biobased 1,5-PDA has been produced in industrial scale by Cathay Industrial Biotech (Shanghai, China) [29]. In addition, Ajinomoto (Tokyo, Japan) is working on the industrial production of biobased 1,5-PDA by decarbonating of lysine via an enzymatic process.
1,8-Octanediamine (1,8-ODA) can be potentially derived from biomass. It can be produced by amination of suberic acid which can be converted from plant oils [118].
1,10-Decanediamine (1,10-DDA) can be chemically converted from sebacic acid derived from castor oils. They are interesting biobased monomers for the synthesis of fully biobased nylon 10,10 which have already been commercially available in the market [31].

Biobased Aromatic Monomers
Lignin is the largest non-carbohydrate components of lignocellulosic biomass which is composed by oxidative coupling of three phenylpropane components: p-coumaryl alcohol, coniferyl alcohol, and sinapyl alcohol [119]. Due to the unique structures and chemical properties, lignin provides a broad opportunity for the production of a wide variety of biobased chemicals, especially biobased aromatic chemicals that so far cannot be accessible via chemical or biological modifications of other biomass feedstocks (Scheme 5).
However, it remains a big challenge to develop an efficient approach for the recovery of aromatic chemicals with tailored structures from lignin [120]. Currently, only vanillin can be produced via a commercial process by oxidation of lignosulfonates, a byproduct from the sulfite pulping industry [121][122][123]. Recently, new chemical and biotechnological approaches for the production of vanillin are studied [23,120,[124][125][126]. Starting from vanillin, many biobased aromatic monomers for polyester synthesis can be produced, for example, vanillic acid, divanillyl diol, dimethyl divanillate, and so on [127][128][129][130][131].
Terephthalic acid (TPA) is industrially produced by oxidation of p-xylene. It is used mainly as a precursor for the production of aromatic polyesters and polyamides such as PET, PBT and PPAs. The current global market size of TPA is around 30 million tons per year, and is expected to increase to 60 million tons in 2020 [31]. Nowadays, several technologies to produce biobased TPA and its precursors from renewable resources have been proposed (Scheme 6) [49,[132][133][134][135][136][137][138][139]; and some companies and research institutes are active in the development of biobased TPA [31,49,138] and full biobased PET. Nevertheless, no commercial biobased TPA and fully biobased PET are current available in the market.
2,5-Furandicarboxylic acid (FDCA) is an interesting biobased rigid monomer, which is considered as the most promising substitute to petrol-based TPA and IPA [5,14,140]. Currently, FDCA is readily produced from biomass feedstocks, for example, by oxidation of HMF derived from various sources of carbohydrates [18,24]. It is also possible to produce FDCA via a biocatalytic approach starting from HMF (Scheme 7) [141]. At present, FDCA is industrially produced by Avantium (The Netherlands) using an enabling chemical synthesis technology [14,31]; and the price is expected to be cheaper than the biobased and petrol-based TPA [31,142].

Other Biobased Monomers
Lactic acid, one of the most well-known organic acids occurring naturally, can be found in many carbohydrates, for example, in naturally and fermented food products, plant, human beings and animals [144]. In most living organisms, lactic acid is also identified as a principal metabolic intermediate. Lactic acid can be manufactured chemically or biologically in industry [144]. In the chemical synthesis approach, lactic acid is prepared via hydrolysis of lactonitrile, a by-product of acrylonitrile production, by concentrated hydrochloric or sulfuric acid. This process is simple, but results in a racemic mixture of D-and L-lactic acid; and the production of lactic acid depends on the acrylonitrile industry in this case [145]. On the other hand, lactic acid can be produced via fermentation of sugars by bacteria. This microbial fermentation process involves the utilization of biomass feedstocks, low reaction temperature, low energy consumption and can resulted in enantiopure lactic acid by selecting an appropriate microbial strain [145][146][147]. Currently, the global demand of lactic acid is 350 kilo ton per year, with a sustainable growth in the next decade; and more than 90% of lactic acid is commercially produced via fermentation of glucose [59]. Alternatively, production of lactic acid from biobased glycerol and its derivatives is feasibly; however, this route cannot compete with the fermentation process because of the high cost.
Many long chain fatty acids and their derivatives can be produced from renewable resources such as plant oils and fats [97,[151][152][153], and they are good building blocks for polyester and polyamide synthesis. Examples of long chain fatty acids include oleic acid, ricinoleic acid, erucic acid, vernolic acid, and so on [9,154].

Other Biobased Monomers
Lactic acid, one of the most well-known organic acids occurring naturally, can be found in many carbohydrates, for example, in naturally and fermented food products, plant, human beings and animals [144]. In most living organisms, lactic acid is also identified as a principal metabolic intermediate. Lactic acid can be manufactured chemically or biologically in industry [144]. In the chemical synthesis approach, lactic acid is prepared via hydrolysis of lactonitrile, a by-product of acrylonitrile production, by concentrated hydrochloric or sulfuric acid. This process is simple, but results in a racemic mixture of D-and L-lactic acid; and the production of lactic acid depends on the acrylonitrile industry in this case [145]. On the other hand, lactic acid can be produced via fermentation of sugars by bacteria. This microbial fermentation process involves the utilization of biomass feedstocks, low reaction temperature, low energy consumption and can resulted in enantio-pure lactic acid by selecting an appropriate microbial strain [145][146][147]. Currently, the global demand of lactic acid is 350 kilo ton per year, with a sustainable growth in the next decade; and more than 90% of lactic acid is commercially produced via fermentation of glucose [59]. Alternatively, production of lactic acid from biobased glycerol and its derivatives is feasibly; however, this route cannot compete with the fermentation process because of the high cost.
Many long chain fatty acids and their derivatives can be produced from renewable resources such as plant oils and fats [97,[151][152][153], and they are good building blocks for polyester and polyamide synthesis. Examples of long chain fatty acids include oleic acid, ricinoleic acid, erucic acid, vernolic acid, and so on [9,154].
It is generally acknowledged that the specificity, selectivity and catalytic reactivity of an enzyme depend on its active site, the region that undergoes the binding of substrate molecules and the occurrence of enzymatic reactions. The active site of an enzyme consists of amino acid residuals that form temporary bonds with the substrate (binding site) and other amino acid residues that catalyze the corresponding reaction of that substrate (catalytic site). As for lipases, the active site is situated inside a pocket, which is located above the central β-sheet of the protein [174]. Although the active sites of lipases have different shapes, sizes, depths of the pockets, and physicochemical characteristics of their amino acids [175], the binding sites display highly homologous amino acid sequences [171]; and the active site of lipases consists of a highly conserved catalytic triad: a nucleophilic residue (serine), a histidine base and a catalytic acidic residue (aspartic or glutamic acid, usually aspartic acid) (Scheme 9). In addition, many lipases exhibit a lid, a surface loop that is a lipophilic α-helical domain in the polypeptide chain and covers the active sites [171,176]. The lid controls the access of substrate molecules to the catalytic center of lipase. In the presence of a lipid-water interface, the lid opens the active center and thus the active site becomes accessible. In this case, a large hydrophobic surface of the enzyme is revealed, which activates the enzyme. However, without the lipid-water interface, the lid is in a closed confirmation. As a consequence, the active center is not accessible and the enzyme is inactive. Generally, lipases possess high catalytic reactivity in nonpolar organic solvents with log P (logarithm of partition coefficient) of more than 1.9 [160][161][162]. Examples of suitable organic solvents for lipases are benzene (2), toluene (2.5), diphenyl ether (4.05), hydrocarbons like cyclohexane (3.2) and n-hexane (3.5), and so on [163]. Lipases also function in some green solvents such as ionic liquids and supercritical CO 2 [164][165][166][167][168].
Despite their different sources and diverse structures, all lipases possess a very similar α/β hydrolase fold (Scheme 9). The α/β hydrolase fold consists of a β-sheet core of five to eight parallel strands (only the second β strand shows an antiparallel orientation to the others) connected on both sides by α-helices, forming a α/β/α sandwich-like shape [169][170][171][172]. Lipases and other enzymes including esterases, proteases, dehalogenases, epoxide hydrolases and peroxidases which exhibit similar structural features, belong to the α/β hydrolase family [169,173].
It is generally acknowledged that the specificity, selectivity and catalytic reactivity of an enzyme depend on its active site, the region that undergoes the binding of substrate molecules and the occurrence of enzymatic reactions. The active site of an enzyme consists of amino acid residuals that form temporary bonds with the substrate (binding site) and other amino acid residues that catalyze the corresponding reaction of that substrate (catalytic site). As for lipases, the active site is situated inside a pocket, which is located above the central β-sheet of the protein [174]. Although the active sites of lipases have different shapes, sizes, depths of the pockets, and physicochemical characteristics of their amino acids [175], the binding sites display highly homologous amino acid sequences [171]; and the active site of lipases consists of a highly conserved catalytic triad: a nucleophilic residue (serine), a histidine base and a catalytic acidic residue (aspartic or glutamic acid, usually aspartic acid) (Scheme 9). In addition, many lipases exhibit a lid, a surface loop that is a lipophilic α-helical domain in the polypeptide chain and covers the active sites [171,176]. The lid controls the access of substrate molecules to the catalytic center of lipase. In the presence of a lipid-water interface, the lid opens the active center and thus the active site becomes accessible. In this case, a large hydrophobic surface of the enzyme is revealed, which activates the enzyme. However, without the lipid-water interface, the lid is in a closed confirmation. As a consequence, the active center is not accessible and the enzyme is inactive. Scheme 9. Secondary structure diagram of the α/β hydrolase fold and the location of catalytic triad amino acid residues in lipases. Ser: serine residue; Asp or Glu: aspartic or glutamic acid residue; His: histidine residue; helixes indicate α-helixes; arrows indicate β-sheets [177].
The general catalytic mechanism of lipases is illustrated in Scheme 10, which involves an acylation step followed by a deacylation step [171,174]. At the acylation step, the hydroxyl group of the catalytic serine is activated by transferring a proton among the aspartate, histidine, and serine residues of the catalytic triad, rendering an increase of the nucleophilicity of the hydroxyl residue of the serine. After that, the hydroxyl residue of the serine attacks the carbonyl group of the substrate (carboxylic ester or carboxylic acid), forming the first tetrahedral intermediate with a negative charge on the oxygen of the carbonyl group. The oxyanion hole is formed by hydrogen bonding between the amide groups of the amino acid residuals of the enzyme and the carbonyl group oxygen of the substrate. By the formation of at least two hydrogen bonds in the oxyanion hole, the charge distribution is stabilized and the state energy of the tetrahedral intermediate is reduced. Then the alcohol component (R1-OH) is released from the bond with the intermediate, while the "acidic component" of the substrate remains covalently bound to the serine residue in the acyl-enzyme intermediate. When the enzyme is attacked by a nucleophile (R2-OH), the deacylation step occurs. The product (a new carboxylic ester or carboxylic acid) is then released, while the enzyme is regenerated. This nucleophile (R2-OH) can be water (hydrolysis) or an alcohol (alcoholysis). To increase the stability towards organic solvents and to facilitate the recycling and reusing, lipases are normally used in their immobilized forms [178][179][180][181][182][183][184][185]. The immobilized lipases may show improved catalytic activity, specificity or selectivity. Similar to other enzymes, lipases can be generally immobilized via three strategies [178]: (1) chemical or physical adsorptions onto an inert matrix; (2) entrapment within an inert matrix; and (3) immobilized as water-insoluble particles: cross-Scheme 9. Secondary structure diagram of the α/β hydrolase fold and the location of catalytic triad amino acid residues in lipases. Ser: serine residue; Asp or Glu: aspartic or glutamic acid residue; His: histidine residue; helixes indicate α-helixes; arrows indicate β-sheets [177].
The general catalytic mechanism of lipases is illustrated in Scheme 10, which involves an acylation step followed by a deacylation step [171,174]. At the acylation step, the hydroxyl group of the catalytic serine is activated by transferring a proton among the aspartate, histidine, and serine residues of the catalytic triad, rendering an increase of the nucleophilicity of the hydroxyl residue of the serine. After that, the hydroxyl residue of the serine attacks the carbonyl group of the substrate (carboxylic ester or carboxylic acid), forming the first tetrahedral intermediate with a negative charge on the oxygen of the carbonyl group. The oxyanion hole is formed by hydrogen bonding between the amide groups of the amino acid residuals of the enzyme and the carbonyl group oxygen of the substrate. By the formation of at least two hydrogen bonds in the oxyanion hole, the charge distribution is stabilized and the state energy of the tetrahedral intermediate is reduced. Then the alcohol component (R 1 -OH) is released from the bond with the intermediate, while the "acidic component" of the substrate remains covalently bound to the serine residue in the acyl-enzyme intermediate. When the enzyme is attacked by a nucleophile (R 2 -OH), the deacylation step occurs. The product (a new carboxylic ester or carboxylic acid) is then released, while the enzyme is regenerated. This nucleophile (R 2 -OH) can be water (hydrolysis) or an alcohol (alcoholysis). The general catalytic mechanism of lipases is illustrated in Scheme 10, which involves an acylation step followed by a deacylation step [171,174]. At the acylation step, the hydroxyl group of the catalytic serine is activated by transferring a proton among the aspartate, histidine, and serine residues of the catalytic triad, rendering an increase of the nucleophilicity of the hydroxyl residue of the serine. After that, the hydroxyl residue of the serine attacks the carbonyl group of the substrate (carboxylic ester or carboxylic acid), forming the first tetrahedral intermediate with a negative charge on the oxygen of the carbonyl group. The oxyanion hole is formed by hydrogen bonding between the amide groups of the amino acid residuals of the enzyme and the carbonyl group oxygen of the substrate. By the formation of at least two hydrogen bonds in the oxyanion hole, the charge distribution is stabilized and the state energy of the tetrahedral intermediate is reduced. Then the alcohol component (R1-OH) is released from the bond with the intermediate, while the "acidic component" of the substrate remains covalently bound to the serine residue in the acyl-enzyme intermediate. When the enzyme is attacked by a nucleophile (R2-OH), the deacylation step occurs. The product (a new carboxylic ester or carboxylic acid) is then released, while the enzyme is regenerated. This nucleophile (R2-OH) can be water (hydrolysis) or an alcohol (alcoholysis).
Due to the broad substrate specificity, high selectivity, and high thermal stability and catalytic reactivity, Candida antarctica lipase b (CALB), which was reclassified as Pseudozyma antarctica lipase b (PALB) more recently [186], is the most popular biocatalyst which is extensively used in biocatalytic synthesis of small molecules and polymers. CALB is a globular protein that is composed of 317 amino acids (Scheme 11), having a molecular weight of 33 kDa. Similar to other lipases, CALB possesses a Ser-His-Asp catalytic triad (Ser105, Asp187 and His224) in its active site and two oxyanion holes (Thr40 and Gln106) [187], and the catalytic mechanism of CALB is the same as other lipases. Due to the broad substrate specificity, high selectivity, and high thermal stability and catalytic reactivity, Candida antarctica lipase b (CALB), which was reclassified as Pseudozyma antarctica lipase b (PALB) more recently [186], is the most popular biocatalyst which is extensively used in biocatalytic synthesis of small molecules and polymers. CALB is a globular protein that is composed of 317 amino acids (Scheme 11), having a molecular weight of 33 kDa. Similar to other lipases, CALB possesses a Ser-His-Asp catalytic triad (Ser105, Asp187 and His224) in its active site and two oxyanion holes (Thr40 and Gln106) [187], and the catalytic mechanism of CALB is the same as other lipases. However, the presence of the lid structure and the interfacial activation of CALB are still under debate. Some literature suggested that the two α-helixes (α5 and α10) surrounding the active center of CALB, the most mobile part of the structure, could work as the lid [188][189][190][191], and CALB is an interfacial activated enzyme. A recent study indicated the hydrophobicity of the interface and the overall size of the substrate determine the interfacial activation of CALB [190], Others suggested that CALB has no lid covering the entrance of the active site [187] and displays no interfacial activation [192]. In addition, CALB has a very limited available space in the pocket of active site compared to other lipases and this explains its high selectivity [193].
N435 is the primary immobilized CALB that is used both in the industrial area and academia research. N435 functions as a hydrophobic biocatalyst, which consists of 10 wt % of CALB physically absorbed within 90 wt % of Lewatit VP OC 1600 bead which is a macroporous DVB-crosslinked methacrylate polymer resin [162,194,195]. The bead size of N435 ranges from 0.315 to 1.0 mm (>80%), the effective size is around 0.32-0.45 mm, and the average pore diameter is 15 nm. N435 can work at mild conditions and especially, can tolerate some extreme conditions such as elevated temperatures (up to 150 °C) [196][197][198].

Enzyme-Catalyzed Synthesis of Polyesters
Enzymatic polymerization is defined as "in vitro (in the test tubes) chemical synthesis of polymers via a non-biosynthetic (non-metabolic) approach using an isolated enzyme as the catalyst" [36,199]. However, the presence of the lid structure and the interfacial activation of CALB are still under debate. Some literature suggested that the two α-helixes (α5 and α10) surrounding the active center of CALB, the most mobile part of the structure, could work as the lid [188][189][190][191], and CALB is an interfacial activated enzyme. A recent study indicated the hydrophobicity of the interface and the overall size of the substrate determine the interfacial activation of CALB [190], Others suggested that CALB has no lid covering the entrance of the active site [187] and displays no interfacial activation [192]. In addition, CALB has a very limited available space in the pocket of active site compared to other lipases and this explains its high selectivity [193].
N435 is the primary immobilized CALB that is used both in the industrial area and academia research. N435 functions as a hydrophobic biocatalyst, which consists of 10 wt % of CALB physically absorbed within 90 wt % of Lewatit VP OC 1600 bead which is a macroporous DVB-crosslinked methacrylate polymer resin [162,194,195]. The bead size of N435 ranges from 0.315 to 1.0 mm (>80%), the effective size is around 0.32-0.45 mm, and the average pore diameter is 15 nm. N435 can work at mild conditions and especially, can tolerate some extreme conditions such as elevated temperatures (up to 150˝C) [196][197][198].

Enzyme-Catalyzed Synthesis of Polyesters
Enzymatic polymerization is defined as "in vitro (in the test tubes) chemical synthesis of polymers via a non-biosynthetic (non-metabolic) approach using an isolated enzyme as the catalyst" [36,199].
Due to the unique properties of enzymes, enzymatic polymerization inherits many merits such as high specificity and selectivity towards monomer substrates, clean-process, energy saving, gentle environmental footprint, nontoxic natural catalysts, and recyclable catalysts (after immobilization). With these, enzymatic polymerization provides an opportunity to achieve "green polymer chemistry".
Among them, polycondensation and ring-opening polymerization are the most common methods used for biocatalytic polyester synthesis.
Four modes of elemental reactions may occur during the lipase-catalyzed polyester synthesis, inducing hydrolysis, esterification, transesterification (alcoholysis and acidolysis), and interesterification (Scheme 13). These reactions are all reversible. Therefore, to facilitate the ester formation, it is crucial to remove the remaining water and byproducts like alcohols from the reaction mixture, for example, by adding absorbing and drying agents like molecular sieves, applying reduced pressure, using azeotropic distillation conditions, and so on.
The first lipase-catalyzed polymerization was reported by Okumara et al. in 1984 [209]. They investigated the enzymatic polymerization of aliphatic diacids and diols by a lipase from Aspergillus niger NRRL 337 (Scheme 14). However, only oligoesters with M n 's of around 1000 g/mol were obtained.
Generally speaking, three polymerization modes can be proceeded for the lipase-catalyzed polyester synthesis (Scheme 12): (1) step-growth polycondensation; (2) ring-opening polymerization; and (3) a combination of ring-opening polymerization and polycondensation (ring-opening additioncondensation polymerization). Among them, polycondensation and ring-opening polymerization are the most common methods used for biocatalytic polyester synthesis. Four modes of elemental reactions may occur during the lipase-catalyzed polyester synthesis, inducing hydrolysis, esterification, transesterification (alcoholysis and acidolysis), and interesterification (Scheme 13). These reactions are all reversible. Therefore, to facilitate the ester formation, it is crucial to remove the remaining water and byproducts like alcohols from the reaction mixture, for example, by adding absorbing and drying agents like molecular sieves, applying reduced pressure, using azeotropic distillation conditions, and so on. The first lipase-catalyzed polymerization was reported by Okumara et al. in 1984 [209]. They investigated the enzymatic polymerization of aliphatic diacids and diols by a lipase from Aspergillus niger NRRL 337 (Scheme 14). However, only oligoesters with 's of around 1000 g/mol were obtained. The lipase-catalyzed ring-opening polymerization was firstly reported in 1993 by two independent groups [210,211]. Gutman et al. [210] investigated the lipase-catalyzed ring-opening polymerization of ε-caprolactone (ε-CL); and polycaprolactone (PCL) with a of up to 4400 g/mol was successfully produced in n-hexane (Scheme 15). At the same time, the enzymatic ring-opening polymerization of lactones was performed in bulk by Kobayashi et al. [211], using different lipases as catalysts. The enzymatic polymerization gave PCL and polyvalerolactone with 's of up to 7700, and 1900 g/mol, respectively. Four modes of elemental reactions may occur during the lipase-catalyzed polyester synthesis, inducing hydrolysis, esterification, transesterification (alcoholysis and acidolysis), and interesterification (Scheme 13). These reactions are all reversible. Therefore, to facilitate the ester formation, it is crucial to remove the remaining water and byproducts like alcohols from the reaction mixture, for example, by adding absorbing and drying agents like molecular sieves, applying reduced pressure, using azeotropic distillation conditions, and so on. The first lipase-catalyzed polymerization was reported by Okumara et al. in 1984 [209]. They investigated the enzymatic polymerization of aliphatic diacids and diols by a lipase from Aspergillus niger NRRL 337 (Scheme 14). However, only oligoesters with 's of around 1000 g/mol were obtained. The lipase-catalyzed ring-opening polymerization was firstly reported in 1993 by two independent groups [210,211]. Gutman et al. [210] investigated the lipase-catalyzed ring-opening polymerization of ε-caprolactone (ε-CL); and polycaprolactone (PCL) with a of up to 4400 g/mol was successfully produced in n-hexane (Scheme 15). At the same time, the enzymatic ring-opening polymerization of lactones was performed in bulk by Kobayashi et al. [211], using different lipases as catalysts. The enzymatic polymerization gave PCL and polyvalerolactone with 's of up to 7700, and 1900 g/mol, respectively. Scheme 15. Lipase-catalyzed ring-opening polymerization of ε-caprolactone. The lipase-catalyzed ring-opening polymerization was firstly reported in 1993 by two independent groups [210,211]. Gutman et al. [210] investigated the lipase-catalyzed ring-opening polymerization of ε-caprolactone (ε-CL); and polycaprolactone (PCL) with a M n of up to 4400 g/mol was successfully produced in n-hexane (Scheme 15). At the same time, the enzymatic ring-opening polymerization of lactones was performed in bulk by Kobayashi et al. [211], using different lipases as catalysts. The enzymatic polymerization gave PCL and polyvalerolactone with M n 's of up to 7700, and 1900 g/mol, respectively. independent groups [210,211]. Gutman et al. [210] investigated the lipase-catalyzed ring-opening polymerization of ε-caprolactone (ε-CL); and polycaprolactone (PCL) with a of up to 4400 g/mol was successfully produced in n-hexane (Scheme 15). At the same time, the enzymatic ring-opening polymerization of lactones was performed in bulk by Kobayashi et al. [211], using different lipases as catalysts. The enzymatic polymerization gave PCL and polyvalerolactone with 's of up to 7700, and 1900 g/mol, respectively. Scheme 15. Lipase-catalyzed ring-opening polymerization of ε-caprolactone.
In the late 1990s, the use of N435 in the enzymatic ring-opening polymerization of lactones was introduced by Gross et al. [212] Since then, N435 became the working horse in biocatalytic polyester synthesis.
In the late 1990s, the use of N435 in the enzymatic ring-opening polymerization of lactones was introduced by Gross et al. [212] Since then, N435 became the working horse in biocatalytic polyester synthesis.
It should be pointed out that the large scale production of aliphatic polyesters via lipase-catalyzed polymerization is feasible. As reported by Binns et al. [215], adipic acid and 1,6-HDO were polymerized by N435 at a multi-kilogram scale, using a two-stage method (Scheme 16). The enzymatic polymerization yielded poly(hexamethylene adipate) with a M w of 16,400 g/mol. They also claimed that the enzymatic production can be scaled up to the pilot plant level (2.0 tons) without undue problems. Besides, poly(hexamethylene adipate) produced from the enzymatic polymerization possesses a lower acid number, higher degree of crystallinity and super crystalline growth rate compared to the conventional counterparts. acetals, are studied for the lipase-catalyzed polymerization. The recent progress in this field is comprehensively summarized in some review articles [35,36,[40][41][42]44,213,214].
It should be pointed out that the large scale production of aliphatic polyesters via lipasecatalyzed polymerization is feasible. As reported by Binns et al. [215], adipic acid and 1,6-HDO were polymerized by N435 at a multi-kilogram scale, using a two-stage method (Scheme 16). The enzymatic polymerization yielded poly(hexamethylene adipate) with a of 16,400 g/mol. They also claimed that the enzymatic production can be scaled up to the pilot plant level (2.0 tons) without undue problems. Besides, poly(hexamethylene adipate) produced from the enzymatic polymerization possesses a lower acid number, higher degree of crystallinity and super crystalline growth rate compared to the conventional counterparts. Moreover, macrolides catalyzed by lipases showed higher polymerizability compared to smaller ring-sized lactones [216]. This is probably because macrolides possess higher rates in the formation of enzyme-activated monomers (acyl-enzyme intermediates). However, reverse tendency was observed from anionic and metal (Zn) catalyzed-ring opening polymerization.
Although a great number of aliphatic polyesters are readily synthesized with high molecular weights via lipase-catalyzed polymerization, only limited amount of semi-aromatic and aromatic polyesters are enzymatically produced [217][218][219][220][221][222][223][224][225][226][227]. This could be mainly due to the high melting temperature (Tm) of semi-aromatic and aromatic polyesters and their low solubility in the reaction media, as well as, the lack of reactivity of aromatic monomers in enzymatic polyesterification [210,228]. However, by using cyclic aromatic oligomers in the lipase-catalyzed polymerization, high molecular weight poly(alkylene terephthalate)s, poly (alkylene isophthalate)s and poly(benzenedimethanol adipate)s were obtained, with 's of up to 107,000 g/mol [229].

Enzyme-Catalyzed Synthesis of Polyamides
Lipases, proteases and other enzymes are capable of catalyzing the formation of amide bonds and therefore, they are suitable enzymes for the in vitro polyamide synthesis [206]. In the following discussion of this section, we focus on the lipase-catalyzed polymerization of synthetic polyamides.
Two basic modes of elemental reactions are commonly used in the biocatalytic polyamide synthesis: directly amidation and transamidation (aminolysis) (Scheme 17). Moreover, macrolides catalyzed by lipases showed higher polymerizability compared to smaller ring-sized lactones [216]. This is probably because macrolides possess higher rates in the formation of enzyme-activated monomers (acyl-enzyme intermediates). However, reverse tendency was observed from anionic and metal (Zn) catalyzed-ring opening polymerization.
Although a great number of aliphatic polyesters are readily synthesized with high molecular weights via lipase-catalyzed polymerization, only limited amount of semi-aromatic and aromatic polyesters are enzymatically produced [217][218][219][220][221][222][223][224][225][226][227]. This could be mainly due to the high melting temperature (T m ) of semi-aromatic and aromatic polyesters and their low solubility in the reaction media, as well as, the lack of reactivity of aromatic monomers in enzymatic polyesterification [210,228]. However, by using cyclic aromatic oligomers in the lipase-catalyzed polymerization, high molecular weight poly(alkylene terephthalate)s, poly (alkylene isophthalate)s and poly(benzenedimethanol adipate)s were obtained, with M w 's of up to 107,000 g/mol [229].

Enzyme-Catalyzed Synthesis of Polyamides
Lipases, proteases and other enzymes are capable of catalyzing the formation of amide bonds and therefore, they are suitable enzymes for the in vitro polyamide synthesis [206]. In the following discussion of this section, we focus on the lipase-catalyzed polymerization of synthetic polyamides.
Two basic modes of elemental reactions are commonly used in the biocatalytic polyamide synthesis: directly amidation and transamidation (aminolysis) (Scheme 17).

Enzyme-Catalyzed Synthesis of Polyamides
Lipases, proteases and other enzymes are capable of catalyzing the formation of amide bonds and therefore, they are suitable enzymes for the in vitro polyamide synthesis [206]. In the following discussion of this section, we focus on the lipase-catalyzed polymerization of synthetic polyamides.
Two basic modes of elemental reactions are commonly used in the biocatalytic polyamide synthesis: directly amidation and transamidation (aminolysis) (Scheme 17). The lipase-catalyzed polymerization of polyamides has not been well studied [208]. This could be attributed mainly to two reasons: (1) the high T m of polyamides, and (2) the poor solubility of polyamides in common organic solvents. On the one hand, polyamides like nylons and TPA-based polyamides are semi-crystalline polymers which normally possess a high T m above 100˝C. At such elevated temperatures, the catalytic reactivity of lipases is significantly decreased due to the occurrence of protein denaturation and deactivation. On the other hand, many polyamides can be only dissolved in some aggressive solvents such as formic acid, concentrated H 2 SO 4 , and trifluoroacetic acid, in which lipases cannot act.
Cheng et al. [230,231] investigated the lipase-catalyzed polymerization of diamines and diesters in bulk (Scheme 18), which resulted in aliphatic polyamides with M w 's of around 3000-15,000 g/mol. This is the first report showing that high molecular weight polyamides can be produced from lipase-catalyzed polymerization. The lipase-catalyzed polymerization of polyamides has not been well studied [208]. This could be attributed mainly to two reasons: (1) the high Tm of polyamides, and (2) the poor solubility of polyamides in common organic solvents. On the one hand, polyamides like nylons and TPA-based polyamides are semi-crystalline polymers which normally possess a high Tm above 100 °C. At such elevated temperatures, the catalytic reactivity of lipases is significantly decreased due to the occurrence of protein denaturation and deactivation. On the other hand, many polyamides can be only dissolved in some aggressive solvents such as formic acid, concentrated H2SO4, and trifluoroacetic acid, in which lipases cannot act.
Cheng et al. [230,231] investigated the lipase-catalyzed polymerization of diamines and diesters in bulk (Scheme 18), which resulted in aliphatic polyamides with 's of around 3000-15,000 g/mol. This is the first report showing that high molecular weight polyamides can be produced from lipasecatalyzed polymerization. The CALB-catalyzed ring-opening polymerization of ε-caprolactam was reported by Kong et al. [232]. They claimed that the enzymatic ring-opening polymerization gave nylon 6 with a high of 212,000 g/mol.
Aliphatic polyamides such as nylon 6,13, nylon 8,13 and nylon 12,13 were synthesized via the N435-catalyzed ring-opening addition-condensation (Scheme 19) [197]. The 's of the resulting nylons were around 5600-8300 g/mol. In our group, enzymatic polymerization of polyamides is one of the focused research area. For example, the enzymatic polymerization of 2-azetidinone was first studied in our laboratory (Scheme 20) [233]. A different mechanism for the enzymatic ring-opening polymerization of β-propiolactam was revealed and a catalytic cycle for the oligomerization of β-lactam that rationalizes the activation The CALB-catalyzed ring-opening polymerization of ε-caprolactam was reported by Kong et al. [232]. They claimed that the enzymatic ring-opening polymerization gave nylon 6 with a high M w of 212,000 g/mol.
The CALB-catalyzed ring-opening polymerization of ε-caprolactam was reported by Kong et al. [232]. They claimed that the enzymatic ring-opening polymerization gave nylon 6 with a high of 212,000 g/mol.
Aliphatic polyamides such as nylon 6,13, nylon 8,13 and nylon 12,13 were synthesized via the N435-catalyzed ring-opening addition-condensation (Scheme 19) [197]. The 's of the resulting nylons were around 5600-8300 g/mol. In our group, enzymatic polymerization of polyamides is one of the focused research area. For example, the enzymatic polymerization of 2-azetidinone was first studied in our laboratory (Scheme 20) [233]. A different mechanism for the enzymatic ring-opening polymerization of β-propiolactam was revealed and a catalytic cycle for the oligomerization of β-lactam that rationalizes the activation of the monomers was proposed [234]. Moreover, aliphatic oligoamides [233,235,236], semi-aromatic oligoamides [237], and poly(ester amide)s [238] are successfully prepared via lipase-catalyzed polymerization in our laboratory. In our group, enzymatic polymerization of polyamides is one of the focused research area. For example, the enzymatic polymerization of 2-azetidinone was first studied in our laboratory (Scheme 20) [233]. A different mechanism for the enzymatic ring-opening polymerization of β-propiolactam was revealed and a catalytic cycle for the oligomerization of β-lactam that rationalizes the activation of the monomers was proposed [234]. Moreover, aliphatic oligoamides [233,235,236], semi-aromatic oligoamides [237], and poly(ester amide)s [238] are successfully prepared via lipase-catalyzed polymerization in our laboratory.
The CALB-catalyzed ring-opening polymerization of ε-caprolactam was reported by Kong et al. [232]. They claimed that the enzymatic ring-opening polymerization gave nylon 6 with a high of 212,000 g/mol.
Aliphatic polyamides such as nylon 6,13, nylon 8,13 and nylon 12,13 were synthesized via the N435-catalyzed ring-opening addition-condensation (Scheme 19) [197]. The 's of the resulting nylons were around 5600-8300 g/mol. In our group, enzymatic polymerization of polyamides is one of the focused research area. For example, the enzymatic polymerization of 2-azetidinone was first studied in our laboratory (Scheme 20) [233]. A different mechanism for the enzymatic ring-opening polymerization of β-propiolactam was revealed and a catalytic cycle for the oligomerization of β-lactam that rationalizes the activation of the monomers was proposed [234]. Moreover, aliphatic oligoamides [233,235,236], semi-aromatic oligoamides [237], and poly(ester amide)s [238] are successfully prepared via lipase-catalyzed polymerization in our laboratory.

Lipase-Catalyzed Synthesis of Sustainable Polyesters and Polyamides from Biobased Monomers
At present, most research on enzymatic polymerization still focused on the use of "traditional" monomers derived from fossil resources. Due to the growing awareness of energy safety and environmental pollution, and increased interest for the development of novel polymeric materials, utilization of biobased monomers in enzymatic polymerization becomes an appealing topic both in the academic and industrial fields. Currently, many (potentially) biobased polyesters and polyamides are readily synthesized via enzymatic polymerization. In this section, the recent developments in the field of the lipase-catalyzed synthesis of biobased polyesters and synthetic polyamides are discussed in details.

Lipase-Catalyzed Synthesis of Sustainable Polyesters and Polyamides from Biobased Monomers
At present, most research on enzymatic polymerization still focused on the use of "traditional" monomers derived from fossil resources. Due to the growing awareness of energy safety and environmental pollution, and increased interest for the development of novel polymeric materials, utilization of biobased monomers in enzymatic polymerization becomes an appealing topic both in the academic and industrial fields. Currently, many (potentially) biobased polyesters and polyamides are readily synthesized via enzymatic polymerization. In this section, the recent developments in the field of the lipase-catalyzed synthesis of biobased polyesters and synthetic polyamides are discussed in details However, the direct enzymatic ring-opening polymerization of lactides generally resulted in PLA with low molecular weights or low reaction yields, indicating that the enzymatic polymerization efficiency was quite low. It was also found that the enzymatic polymerization of D,L-lactide resulted in higher molecular weight products compared to D,D-and L,L-lactide [239][240][241]. Nevertheless, after However, the direct enzymatic ring-opening polymerization of lactides generally resulted in PLA with low molecular weights or low reaction yields, indicating that the enzymatic polymerization efficiency was quite low. It was also found that the enzymatic polymerization of D,L-lactide resulted in higher molecular weight products compared to D,D-and L,L-lactide [239][240][241]. Nevertheless, after careful adjusting the reaction conditions, high molecular weight poly(D,D-lactide) (PDLA) can be synthesized from the N435-catalyzed ring-opening polymerization, with a M n , dispersity and conversion of 12,000 g/mol, 1.1 and 60%, respectively [242]. In addition, poly(L,L-lactide) (PLLA) can be produced from the N435-catalyzed ring-opening polymerization in supercritical CO 2 [243]. Although the resulting PLLA possessed a high M w (12,900 g/mol) and a good dispersity (around 1.2), the reaction yield was quite low, less than 12%.
A new biocatalytic approach was developed for the efficient synthesis of high molecular weight PLLA and PDLA, starting from an O-carboxylic anhydride derived from lactic acid (L-or D-lacOCA) (Scheme 22) [244]. The M n , dispersity and reaction yield of the resulting PLLA and PDLA were up to 38,400 g/mol, ď1.4, and around 90%, respectively. In addition, the tested lipases showed slight preference to L-lacOCA over D-lacOCA. Moreover, the molecular weights of the obtained PLLA can be controllable by altering the concentration of N435 in the reaction media. Moreover, many PLA co-polyesters were successfully synthesized via lipase-catalyzed copolymerization, including poly(lactide-co-trimethylene carbonate) [246], poly(lactide-co-glycolide) [247], and poly(lactide-co-alkylene dicarboxylate) [248] (Scheme 23). The corresponding 's were around 12,000-21,000, 2200-20,600, and 10,000-38,000 g/mol, respectively. Besides, the obtained copolyesters can be optically active, due to the retention of the chiral configuration of lactate units after the enzymatic polymerization [248]. PBS is normally synthesized via polycondensation of succinic acid or succinic anhydride with 1,4-BDO at elevated temperatures, using a chemical catalyst [249]. It is also promising to synthesize biobased PBS via enzymatic polymerization.
The lipase-catalyzed polycondensation of PBS was studied by Gross et al. [250], using a twostage method which is similar to those used for the industrial production but at much lower temperatures (Scheme 24). The solvent-free enzymatic polycondensation with succinic acid gave oligomers. However, by replacing succinic acid with diethyl succinate, the temperature varied two-  [245]. The enzymatic polymerization yielded PLAs with M n 's and dispersities of around 1500-36,700 g/mol, and 1.0-1.5, respectively.
The lipase-catalyzed polycondensation of PBS was studied by Gross et al. [250], using a two-stage method which is similar to those used for the industrial production but at much lower temperatures (Scheme 24). The solvent-free enzymatic polycondensation with succinic acid gave oligomers. However, by replacing succinic acid with diethyl succinate, the temperature varied two-stage method in diphenyl ether resulted in PBS with a M w of 38,000 g/mol and a dispersity of 1.39. To synthesize PBS with higher molecular weights, another two enzymatic strategies were developed: (1) using cyclic oligomers [251]; and (2) co-polymerization of succinic acid and 1,4-BDO with succinate anhydride [252]. By using cyclic butylene succinate oligomers in the N435-catalyzed polymerization, PBS with a of up to 130,000 g/mol and a dispersity of 1.6 was obtained. However, under similar reaction conditions, the direct enzymatic polycondensation gave PBS with a lower (45,000 g/mol) and a broader dispersity (3.7) (Scheme 25). On the other hand, the enzymatic co-polymerization of succinic acid and 1,4-BDO with succinate anhydride resulted in PBS with a of 73,000 g/mol and a dispersity of 1.7 (Scheme 26). However, although high molecular weight PBS can be enzymatically produced via these two approaches, an extra synthesis step is required. The lipase-catalyzed solvent-free polycondensation of aliphatic diacids (C2-C12) and aliphatic Scheme 24. Enzymatic polycondensation of succinic acid or diethyl succinate and 1,4-butanediol, using a two-stage method [250].
To synthesize PBS with higher molecular weights, another two enzymatic strategies were developed: (1) using cyclic oligomers [251]; and (2) co-polymerization of succinic acid and 1,4-BDO with succinate anhydride [252]. By using cyclic butylene succinate oligomers in the N435-catalyzed polymerization, PBS with a M w of up to 130,000 g/mol and a dispersity of 1.6 was obtained. However, under similar reaction conditions, the direct enzymatic polycondensation gave PBS with a lower M w (45,000 g/mol) and a broader dispersity (3.7) (Scheme 25). On the other hand, the enzymatic co-polymerization of succinic acid and 1,4-BDO with succinate anhydride resulted in PBS with a M w of 73,000 g/mol and a dispersity of 1.7 (Scheme 26). However, although high molecular weight PBS can be enzymatically produced via these two approaches, an extra synthesis step is required. To synthesize PBS with higher molecular weights, another two enzymatic strategies were developed: (1) using cyclic oligomers [251]; and (2) co-polymerization of succinic acid and 1,4-BDO with succinate anhydride [252]. By using cyclic butylene succinate oligomers in the N435-catalyzed polymerization, PBS with a of up to 130,000 g/mol and a dispersity of 1.6 was obtained. However, under similar reaction conditions, the direct enzymatic polycondensation gave PBS with a lower (45,000 g/mol) and a broader dispersity (3.7) (Scheme 25). On the other hand, the enzymatic co-polymerization of succinic acid and 1,4-BDO with succinate anhydride resulted in PBS with a of 73,000 g/mol and a dispersity of 1.7 (Scheme 26). However, although high molecular weight PBS can be enzymatically produced via these two approaches, an extra synthesis step is required. To synthesize PBS with higher molecular weights, another two enzymatic strategies were developed: (1) using cyclic oligomers [251]; and (2) co-polymerization of succinic acid and 1,4-BDO with succinate anhydride [252]. By using cyclic butylene succinate oligomers in the N435-catalyzed polymerization, PBS with a of up to 130,000 g/mol and a dispersity of 1.6 was obtained. However, under similar reaction conditions, the direct enzymatic polycondensation gave PBS with a lower (45,000 g/mol) and a broader dispersity (3.7) (Scheme 25). On the other hand, the enzymatic co-polymerization of succinic acid and 1,4-BDO with succinate anhydride resulted in PBS with a of 73,000 g/mol and a dispersity of 1.7 (Scheme 26). However, although high molecular weight PBS can be enzymatically produced via these two approaches, an extra synthesis step is required.

Other Biobased Aliphatic Polyesters
Many other (potential) biobased aliphatic polyesters are synthesized via lipase-catalyzed polycondensation. Some examples are discussed as follows.
The lipase-catalyzed polymerization of aliphatic diacid ethyl esters (C2, C4 and C8) and diols (C4, C6 and C8) were performed in bulk or by using β-cyclodextrin as the support architecture. Various saturated aliphatic polyesters were produced, with 's ranging from 5300 to 44,600 g/mol [255,256].
Recently, we succeeded in preparing a series of (potentially) biobased poly(butylene dicarboxylate)s via the N435-catalyzed polycondensation of 1,4-butanediol and diacid ethyl esters differing in chain length (C2, C3, C4, C6, C8 and C10) (Scheme 28) [257]. High molecular weight poly(butylene dicarboxylate)s were obtained, with 's of up to 94,000 g/mol. We found that increasing the chain length of diacid ethyl ester from C2 to C4 resulted in poly(butylene dicarboxylate)s of significant higher molecular weights; however, upon further increasing the chain length from C4 to C10, poly(butylene dicarboxylate)s with lower molecular weights were obtained. Meanwhile, the enzymatic polymerization with diethyl succinate (C2) gave the lowest molecular weight products. This suggested that CALB possesses a higher selectivity towards diacid ethyl esters with a >C2 chain length; and CALB prefers diethyl adipate (C4) over the other tested counterparts. Scheme 28. Enzymatic synthesis of poly(butylene dicarboxylate)s via N435-catalyzed polycondensation of 1,4-butanediol and diacid ethyl esters differing in chain length [257].
The lipase-catalyzed polymerization of aliphatic diacid ethyl esters (C2, C4 and C8) and diols (C4, C6 and C8) were performed in bulk or by using β-cyclodextrin as the support architecture. Various saturated aliphatic polyesters were produced, with M w 's ranging from 5300 to 44,600 g/mol [255,256].
The lipase-catalyzed polymerization of aliphatic diacid ethyl esters (C2, C4 and C8) and diols (C4, C6 and C8) were performed in bulk or by using β-cyclodextrin as the support architecture. Various saturated aliphatic polyesters were produced, with 's ranging from 5300 to 44,600 g/mol [255,256].
Recently, we succeeded in preparing a series of (potentially) biobased poly(butylene dicarboxylate)s via the N435-catalyzed polycondensation of 1,4-butanediol and diacid ethyl esters differing in chain length (C2, C3, C4, C6, C8 and C10) (Scheme 28) [257]. High molecular weight poly(butylene dicarboxylate)s were obtained, with 's of up to 94,000 g/mol. We found that increasing the chain length of diacid ethyl ester from C2 to C4 resulted in poly(butylene dicarboxylate)s of significant higher molecular weights; however, upon further increasing the chain length from C4 to C10, poly(butylene dicarboxylate)s with lower molecular weights were obtained. Meanwhile, the enzymatic polymerization with diethyl succinate (C2) gave the lowest molecular weight products. This suggested that CALB possesses a higher selectivity towards diacid ethyl esters with a >C2 chain length; and CALB prefers diethyl adipate (C4) over the other tested counterparts. Scheme 28. Enzymatic synthesis of poly(butylene dicarboxylate)s via N435-catalyzed polycondensation of 1,4-butanediol and diacid ethyl esters differing in chain length [257].

Biobased Unsaturated Aliphatic Polyesters
Currently, the synthesis of biobased unsaturated polyesters, especially itaconate-based unsaturated polyesters, has not been well studied. This is because the sensitive C=C bond can be deteriorated easily under conventional polymerization conditions such as elevated temperatures and metal catalysts. However, this problem can be easily overcome by using enzyme catalysts in the polymerization, due to the mild synthetic conditions and the high catalytic specificity of the enzyme catalysts.
However, the lipase-catalyzed direct polycondensation of itaconate and aliphatic diols with short chain length generally resulted in oligomers. As reported by Gardossi et al., the solvent-free polyesterification of dimethyl itaconate and 1,4-BDO catalyzed by CALB gave a mixture of oligomers from dimer to pentamer [259,260]. Similarly, the N435-catalyzed polymerization of itaconic anhydride with aliphatic diols (C4-C10) gave oligomers with M n 's of around 150-390 g/mol, although itaconic anhydride was completely consumed [261]. This is because the enzymatic polycondensation is hampered by the low reactivity of itaconate due to the lower electrophilicity of the acyl carbon (C s , Scheme 29) adjacent to the vinyl group [259]. However, the low reactivity of itaconate in enzymatic polymerization could be overcome by optimizing the reaction conditions: (1) improving the mass transfer and the enzyme distribution in the reaction mixture; (2) increasing the enzyme loading; (3) lowering the diol concentration; and (4) choosing more appropriate diols [259]. Currently, the synthesis of biobased unsaturated polyesters, especially itaconate-based unsaturated polyesters, has not been well studied. This is because the sensitive C=C bond can be deteriorated easily under conventional polymerization conditions such as elevated temperatures and metal catalysts. However, this problem can be easily overcome by using enzyme catalysts in the polymerization, due to the mild synthetic conditions and the high catalytic specificity of the enzyme catalysts.
However, the lipase-catalyzed direct polycondensation of itaconate and aliphatic diols with short chain length generally resulted in oligomers. As reported by Gardossi et al., the solvent-free polyesterification of dimethyl itaconate and 1,4-BDO catalyzed by CALB gave a mixture of oligomers from dimer to pentamer [259,260]. Similarly, the N435-catalyzed polymerization of itaconic anhydride with aliphatic diols (C4-C10) gave oligomers with 's of around 150-390 g/mol, although itaconic anhydride was completely consumed [261]. This is because the enzymatic polycondensation is hampered by the low reactivity of itaconate due to the lower electrophilicity of the acyl carbon (Cs, Scheme 29) adjacent to the vinyl group [259]. However, the low reactivity of itaconate in enzymatic polymerization could be overcome by optimizing the reaction conditions: (1) improving the mass transfer and the enzyme distribution in the reaction mixture; (2) increasing the enzyme loading; (3) lowering the diol concentration; and (4) choosing more appropriate diols [259]. Indeed, by using glycols with longer chain lengths or with a rigid structure, itaconate-based homo-polyesters with relatively higher molecular weights were obtained from the lipase-catalyzed polycondensation. As reported by Yousaf et al. [262], the N435-catalyzed polymerization of itaconic acid with 1,4-cyclohexanedimethanol/poly(ethylene glycol) gave homo-polymers with a of 2600 and 8600 g/mol, respectively. On the contrary, the tin(II) 2-ethylhexanoate-catalyzed polycondensation with itaconic acid gelled within hours.
In addition, itaconate-based co-polyesters with high molecular weights can be prepared via lipase-catalyzed co-polymerization, as discussed below.
The N435-catalyzed co-polymerization of itaconic acid, adipic acid and 3-methyl-1,5-pentanediol resulted in a co-polymer with a of 19,000 g/mol [262]. Poly(12-hydroxystearate-co-butylene itaconate) with a of 30,000 g/mol was obtained from the lipase-catalyzed directly polycondensation of methyl 12-hydroxystearate, dimethyl itaconate and 1,4-BDO (Scheme 30) [263]. Moreover, the lipase-catalyzed ring-opening addition-condensation polymerization of methyl 12-hydroxystearate and cyclic butylene itaconate dimer resulted in poly(12hydroxystearate-co-butylene itaconate) with a significantly higher of 160,000 g/mol. Furthermore, the NMR study indicated that the enzymatic polymerization catalyzed by different lipases yielded poly(12-hydroxystearate-co-butylene itaconate) with different microstructures. As shown in Scheme 30, no ester bond was formed between the hydroxyl group of 12-hydroxystearate and the carboxyl group of itaconate when the polymerization was catalyzed by N435. However, by using immobilized Burkholderia cepacia lipase (lipase BC), an ester bond was formed between the 12hydroxystearate and itaconate unit.
Indeed, by using glycols with longer chain lengths or with a rigid structure, itaconate-based homo-polyesters with relatively higher molecular weights were obtained from the lipase-catalyzed polycondensation. As reported by Yousaf et al. [262], the N435-catalyzed polymerization of itaconic acid with 1,4-cyclohexanedimethanol/poly(ethylene glycol) gave homo-polymers with a M w of 2600 and 8600 g/mol, respectively. On the contrary, the tin(II) 2-ethylhexanoate-catalyzed polycondensation with itaconic acid gelled within hours.
In addition, itaconate-based co-polyesters with high molecular weights can be prepared via lipase-catalyzed co-polymerization, as discussed below.
Poly(12-hydroxystearate-co-butylene itaconate) with a M w of 30,000 g/mol was obtained from the lipase-catalyzed directly polycondensation of methyl 12-hydroxystearate, dimethyl itaconate and 1,4-BDO (Scheme 30) [263]. Moreover, the lipase-catalyzed ring-opening addition-condensation polymerization of methyl 12-hydroxystearate and cyclic butylene itaconate dimer resulted in poly(12-hydroxystearate-co-butylene itaconate) with a significantly higher M w of 160,000 g/mol. Furthermore, the NMR study indicated that the enzymatic polymerization catalyzed by different lipases yielded poly(12-hydroxystearate-co-butylene itaconate) with different microstructures. As shown in Scheme 30, no ester bond was formed between the hydroxyl group of 12-hydroxystearate and the carboxyl group of itaconate when the polymerization was catalyzed by N435. However, by using immobilized Burkholderia cepacia lipase (lipase BC), an ester bond was formed between the 12-hydroxystearate and itaconate unit.
compositions ; (2) high molecular weight PBSIs with <30 mol % of itaconate can be prepared by using the two-stage enzymatic polymerization in diphenyl ether; and (3) the two-stage enzymatic melt polymerization gives PBSIs with controllable chemical compositions but low molecular weights. Moreover, the 13 C-NMR study revealed that different microstructures are present in PBSIs obtained from different polymerization methods. The formation of I-B-I-3 microstructures is crucial for synthesizing high molecular weight PBSIs with desired chemical compositions; and more I-B-I-3 microstructures can be produced by CALB in the solvent mixture of cyclohexane and toluene under an azeotropic condition.

Scheme 30.
Lipase-catalyzed synthesis of poly(12-hydroxystearate-co-butylene itaconate), using N435 or immobilized Burkholderia cepacia lipase (lipase BC) as the catalyst. Recently, we investigated the N435-catalyzed polymerization of fully biobased poly(butylene succinate-co-itaconate) (PBSI) (Scheme 31) [264,265]. We found that the enzymatic polycondensation of succinic acid, itaconic acid, and 1,4-butanediol only yielded oligomers, with M w 's of around 500-1500 g/mol, despite different polymerization methods were used. By replacing the unactivated dicarboxylic acids with alkyl diesters, a series of PBSIs with various molar compositions and significant higher molecular weights were obtained, with M w 's of up to 28,300 g/mol. In addition, we found that: (1) the most suitable approach is azeotropic polymerization using the solvent mixture of cyclohexane and toluene, which results in PBSIs with high molecular weights and desirable chemical compositions; (2) high molecular weight PBSIs with <30 mol % of itaconate can be prepared by using the two-stage enzymatic polymerization in diphenyl ether; and (3) the two-stage enzymatic melt polymerization gives PBSIs with controllable chemical compositions but low molecular weights. Moreover, the 13 C-NMR study revealed that different microstructures are present in PBSIs obtained from different polymerization methods. The formation of I-B-I-3 microstructures is crucial for synthesizing high molecular weight PBSIs with desired chemical compositions; and more I-B-I-3 microstructures can be produced by CALB in the solvent mixture of cyclohexane and toluene under an azeotropic condition.
However, by replacing diethyl succinate (C2) with the other diacid ethyl esters with relatively longer chain length (C3~C10), the two-stage enzymatic polymerization in diphenyl ether resulted in series of unsaturated aliphatic polyesters with desired molar compositions and high M w 's of up to 57,900 g/mol (Scheme 32) [257]. The molar percentage of itaconate in the unsaturated polyesters can be tailored from 0% to 35% by adjusting the feed ratio of itaconate; and all C=C bonds were well preserved in the resulting polyesters. We found that products with relatively lower molecular weights were generally obtained from the enzymatic polymerization at a higher feed ratio of itaconate; however, with diethyl dodecanedioate having the longest chain length (C10) among the tested diacid ethyl esters, higher molecular weight products were obtained at higher feed ratios of itaconate. Moreover, the obtained itaconate-based polyesters can be thermally cross-linked or photo-cured. By adjusting the diacid chain length and itaconate composition, the thermal and mechanical properties of the cured polyesters can be tuned.

Scheme 31.
N435-catalyzed synthesis of poly(butylene succinate-co-itaconate) and the corresponding microstructures. However, by replacing diethyl succinate (C2) with the other diacid ethyl esters with relatively longer chain length (C3~C10), the two-stage enzymatic polymerization in diphenyl ether resulted in series of unsaturated aliphatic polyesters with desired molar compositions and high 's of up to 57,900 g/mol (Scheme 32) [257]. The molar percentage of itaconate in the unsaturated polyesters can be tailored from 0% to 35% by adjusting the feed ratio of itaconate; and all C=C bonds were well preserved in the resulting polyesters. We found that products with relatively lower molecular weights were generally obtained from the enzymatic polymerization at a higher feed ratio of itaconate; however, with diethyl dodecanedioate having the longest chain length (C10) among the tested diacid ethyl esters, higher molecular weight products were obtained at higher feed ratios of itaconate. Moreover, the obtained itaconate-based polyesters can be thermally cross-linked or photocured. By adjusting the diacid chain length and itaconate composition, the thermal and mechanical properties of the cured polyesters can be tuned.

Polyesters Derived from Long Chain Fatty Acids and their Derivatives
Long chain fatty acids may contain one or more C=C bonds within the backbones. The C=C bonds can be further modified to form other functional groups such as epoxy, thiol, and hydroxyl group [153,266], rendering fatty acid-based polyesters with diverse functionalities. Fatty acid-based polyesters can be used as thermoset resins, coating materials and biomaterials for biomedical applications, and so on [267][268][269].
The pioneer work on the enzymatic polymerization with long chain fatty acids was reported by Matsumura et al. [270]. They investigated the lipase-catalyzed polymerization of ricinoleic acid/methyl ricinoleate in bulk (Scheme 33). Among the tested lipases, immobilized lipase PC showed the highest reactivity towards ricinoleic acid and methyl ricinoleate. The enzymatic polymerization with ricinoleic acid resulted in polyricinoleate with a of up to 8500 g/mol. However, by replacing ricinoleic acid with methyl ricinoleate, polyricinoleate with a much higher of up to 100,600 g/mol were produced. Scheme 33. Lipase-catalyzed synthesis of polyricinoleate in bulk [270].

Polyesters Derived from Long Chain Fatty Acids and their Derivatives
Long chain fatty acids may contain one or more C=C bonds within the backbones. The C=C bonds can be further modified to form other functional groups such as epoxy, thiol, and hydroxyl group [153,266], rendering fatty acid-based polyesters with diverse functionalities. Fatty acid-based polyesters can be used as thermoset resins, coating materials and biomaterials for biomedical applications, and so on [267][268][269].
The pioneer work on the enzymatic polymerization with long chain fatty acids was reported by Matsumura et al. [270]. They investigated the lipase-catalyzed polymerization of ricinoleic acid/methyl ricinoleate in bulk (Scheme 33). Among the tested lipases, immobilized lipase PC showed the highest reactivity towards ricinoleic acid and methyl ricinoleate. The enzymatic polymerization with ricinoleic acid resulted in polyricinoleate with a M w of up to 8500 g/mol. However, by replacing ricinoleic acid with methyl ricinoleate, polyricinoleate with a much higher M w of up to 100,600 g/mol were produced.
Later, the N435-catalyzed synthesis of poly(12-hydroxydodecanoate-co-12-hydroxystearate) was studied by the same research group (Scheme 34) [271]. The M w , dispersity and reaction yield of the resulting co-polyesters were around 92,300-118,200 g/mol, 2.8-3.3, and 83%-88%, respectively. In addition, the molar percentage of 12-hydroxydodecanoate units in the final products can be tailored from 0% to 100% by adjusting the feed ratio.
The pioneer work on the enzymatic polymerization with long chain fatty acids was reported by Matsumura et al. [270]. They investigated the lipase-catalyzed polymerization of ricinoleic acid/methyl ricinoleate in bulk (Scheme 33). Among the tested lipases, immobilized lipase PC showed the highest reactivity towards ricinoleic acid and methyl ricinoleate. The enzymatic polymerization with ricinoleic acid resulted in polyricinoleate with a of up to 8500 g/mol. However, by replacing ricinoleic acid with methyl ricinoleate, polyricinoleate with a much higher of up to 100,600 g/mol were produced. Scheme 33. Lipase-catalyzed synthesis of polyricinoleate in bulk [270].
On the other hand, cutin and suberin are lipophilic macromolecules which are natural substances found in cell walls of higher plants as structural components. Cutin covers all the aerial surfaces of plants in the plant cuticle, while suberin is the main constituent of cork cells. Their fatty acid derivatives, such as long chain ω-hydroxyalkanoic acids, and α,ω-alkanedioic acids, and
On the other hand, cutin and suberin are lipophilic macromolecules which are natural substances found in cell walls of higher plants as structural components. Cutin covers all the aerial surfaces of plants in the plant cuticle, while suberin is the main constituent of cork cells. Their fatty acid derivatives, such as long chain ω-hydroxyalkanoic acids, and α,ω-alkanedioic acids, and Scheme 36. A two-step biocatalytic synthesis of biobased functional polyesters from ω-carboxy fatty acids and diols [273].
On the other hand, cutin and suberin are lipophilic macromolecules which are natural substances found in cell walls of higher plants as structural components. Cutin covers all the aerial surfaces of plants in the plant cuticle, while suberin is the main constituent of cork cells. Their fatty acid derivatives, such as long chain ω-hydroxyalkanoic acids, and α,ω-alkanedioic acids, and substituted ω-hydroxyalkanoic acids, are attractive biobased monomers for the synthesis of functional aliphatic polyesters [152,274].
Iversen et al. [275] did pioneer work on the enzymatic synthesis of suberin-based polyesters (Scheme 37). The N435-catalyzed polymerization with cis-9,10-epoxy-18-hydroxyoctadecanoic acid in toluene resulted in epoxy-functionalized polyesters with the highest molecular weights. The M w and dispersity were 20,000 g/mol, and 2.2, respectively. In addition, even at a much shorter reaction time of 3 h, the solvent-free enzymatic polymerization in an open vial without any drying agents gave comparable high molecular weights products, with a M w and a dispersity of 15,000 g/mol and 2.2, respectively. substituted ω-hydroxyalkanoic acids, are attractive biobased monomers for the synthesis of functional aliphatic polyesters [152,274]. Iversen et al. [275] did pioneer work on the enzymatic synthesis of suberin-based polyesters (Scheme 37). The N435-catalyzed polymerization with cis-9,10-epoxy-18-hydroxyoctadecanoic acid in toluene resulted in epoxy-functionalized polyesters with the highest molecular weights. The and dispersity were 20,000 g/mol, and 2.2, respectively. In addition, even at a much shorter reaction time of 3 h, the solvent-free enzymatic polymerization in an open vial without any drying agents gave comparable high molecular weights products, with a and a dispersity of 15,000 g/mol and 2.2, respectively. Recently, multifunctional, bio-based oligoester resins based on 9,10-epoxy-18hydroxyoctadecanoic acid were enzymatically synthesized by using N435 as the catalysts (Scheme 38) [276,277]. The , dispersity, monomer conversion and reaction yield of the resulting oligoesters were around 900-1100 g/mol, 2.3-3.1, 95%-99%, and 82%-89%, respectively. Moreover, the functional end groups and the epoxy groups were well preserved after the enzymatic polymerization. The obtained oligoesters can undergo further modifications via different techniques such as Diels-Alder reactions, radical polymerization and ring-opening polymerization. Recently, multifunctional, bio-based oligoester resins based on 9,10-epoxy-18hydroxyoctadecanoic acid were enzymatically synthesized by using N435 as the catalysts (Scheme 38) [276,277]. The M n , dispersity, monomer conversion and reaction yield of the resulting oligoesters were around 900-1100 g/mol, 2.3-3.1, 95%-99%, and 82%-89%, respectively. Moreover, the functional end groups and the epoxy groups were well preserved after the enzymatic polymerization. The obtained oligoesters can undergo further modifications via different techniques such as Diels-Alder reactions, radical polymerization and ring-opening polymerization. substituted ω-hydroxyalkanoic acids, are attractive biobased monomers for the synthesis of functional aliphatic polyesters [152,274].
Iversen et al. [275] did pioneer work on the enzymatic synthesis of suberin-based polyesters (Scheme 37). The N435-catalyzed polymerization with cis-9,10-epoxy-18-hydroxyoctadecanoic acid in toluene resulted in epoxy-functionalized polyesters with the highest molecular weights. The and dispersity were 20,000 g/mol, and 2.2, respectively. In addition, even at a much shorter reaction time of 3 h, the solvent-free enzymatic polymerization in an open vial without any drying agents gave comparable high molecular weights products, with a and a dispersity of 15,000 g/mol and 2.2, respectively. Recently, multifunctional, bio-based oligoester resins based on 9,10-epoxy-18hydroxyoctadecanoic acid were enzymatically synthesized by using N435 as the catalysts (Scheme 38) [276,277]. The , dispersity, monomer conversion and reaction yield of the resulting oligoesters were around 900-1100 g/mol, 2.3-3.1, 95%-99%, and 82%-89%, respectively. Moreover, the functional end groups and the epoxy groups were well preserved after the enzymatic polymerization. The obtained oligoesters can undergo further modifications via different techniques such as Diels-Alder reactions, radical polymerization and ring-opening polymerization. Scheme 38. N435-catalyzed synthesis of bio-based oligoesters based on 9,10-epoxy-18hydroxyoctadecanoic acid.

Glycerol-Based Polyesters
Glycerol-based aliphatic polyesters can be used as thermosets like shape memory materials; and have found potential applications in biomedical and pharmaceutical fields, for example, they can be used as carriers for drug delivery, sealants or coatings for tissue repair, and agents for antibacterial applications [278].
The N435-catalyzed polymerization of divinyl adipate and glycerol in bulk yielded poly(glyceryl adipate) with a M w and dispersity of up to 10,400 g/mol and 2.3-3.1, respectively (Scheme 39) [279]. MALDI-ToF MS analysis suggested that linear polyesters with hydroxyl substituents were mainly produced and no polymer network was formed. The number of hydroxyl groups per repeating units was around 0.8-0.9; and the pendant groups of the synthetic poly(glyceryl adipate) consisted of 90%-95% of secondary and 5%-10% of primary hydroxyl groups.

Glycerol-Based Polyesters
Glycerol-based aliphatic polyesters can be used as thermosets like shape memory materials; and have found potential applications in biomedical and pharmaceutical fields, for example, they can be used as carriers for drug delivery, sealants or coatings for tissue repair, and agents for antibacterial applications [278].
The N435-catalyzed polymerization of divinyl adipate and glycerol in bulk yielded poly(glyceryl adipate) with a and dispersity of up to 10,400 g/mol and 2.3-3.1, respectively (Scheme 39) [279]. MALDI-ToF MS analysis suggested that linear polyesters with hydroxyl substituents were mainly produced and no polymer network was formed. The number of hydroxyl groups per repeating units was around 0.8-0.9; and the pendant groups of the synthetic poly(glyceryl adipate) consisted of 90%-95% of secondary and 5%-10% of primary hydroxyl groups. Scheme 39. N435-catalyzed polymerization of divinyl adipate and glycerol with or without 1,4butanediol in bulk [279].
By replacing the activated divinyl adipate with unactivated adipic acid, the N435-catalyzed enzymatic polycondensation also resulted in poly(glyceryl adipate), with a slight low M w of 3700 g/mol and a dispersity of 1.4 (Scheme 40) [280].

Glycerol-Based Polyesters
Glycerol-based aliphatic polyesters can be used as thermosets like shape memory materials; and have found potential applications in biomedical and pharmaceutical fields, for example, they can be used as carriers for drug delivery, sealants or coatings for tissue repair, and agents for antibacterial applications [278].
The N435-catalyzed polymerization of divinyl adipate and glycerol in bulk yielded poly(glyceryl adipate) with a and dispersity of up to 10,400 g/mol and 2.3-3.1, respectively (Scheme 39) [279]. MALDI-ToF MS analysis suggested that linear polyesters with hydroxyl substituents were mainly produced and no polymer network was formed. The number of hydroxyl groups per repeating units was around 0.8-0.9; and the pendant groups of the synthetic poly(glyceryl adipate) consisted of 90%-95% of secondary and 5%-10% of primary hydroxyl groups. Scheme 39. N435-catalyzed polymerization of divinyl adipate and glycerol with or without 1,4butanediol in bulk [279].
At a molar monomer feed ratio of 1.0:1.0, the M n and dispersity of the obtained polyesters were up to 9100 g/mol, and around 3.3-3.4, respectively. However, the percentage of dendritic glycerol units (Den %) was quite low, around 13%-16%. By increasing the molar feed ratio of oleic diacid and glycerol from 1.0:1.0 to 1.0:1.5, the resulting polyesters possessed a similar M n and dispersity, but a significant higher Den % (~31%). In contrast, gelation was observed in the polymerization catalyzed by dibutyltin oxide. Moreover, several glycerol-based co-polyesters were successfully produced via lipase-catalyzed polycondensation.
The enzymatic co-polymerization of divinyl adipate, glycerol and 1,4-BDO gave poly(glyceryl adipate-co-butylene adipate) (Scheme 39) [279]. The hydroxyl number of the obtained co-polyesters can be well controlled by adjusting the amount of 1,4-BDO in the reaction mixture.
Poly(octamethylene adipate-co-glyceryl adipate) were successfully produced via the N435catalyzed co-polymerization of glycerol, adipic acid and 1,8-octanediol in bulk (Scheme 40) [280][281][282], with 's of up to 75,600 g/mol. The 13 C-NMR study indicated that the obtained polyesters were highly branched but had few interchain cross-links; and the degree of branching and molecular weights can be controlled by altering the reaction time and molar feed ratio of monomers [282]. In addition, due to the regio-selectivity of N435, the enzymatic polymerization gave linear polyesters at short reaction times (≤18 h) but yielded highly branched polyesters at a long reaction time (42 h). Moreover, with respect to esterifications, N435 showed 77% to 82% of the regio-selectivity towards the primary hydroxyl groups of glycerol and this was independent of the amount of glycerol in the reaction media.
The enzymatic co-polymerization of divinyl esters, glycerol and ω-fatty acids were also investigated, using lipases as biocatalysts (Scheme 42) [284,285]. Among the tested lipases, N435 showed the highest catalytic activity. The enzymatic polymerization yielded biodegradable crosslinkable polyesters with 's of up to 8500 g/mol. The obtained polyesters were thermally crosslinked, which resulted in transparent polymeric films with high-gloss surfaces.
The enzymatic co-polymerization of divinyl adipate, glycerol and 1,4-BDO gave poly(glyceryl adipate-co-butylene adipate) (Scheme 39) [279]. The hydroxyl number of the obtained co-polyesters can be well controlled by adjusting the amount of 1,4-BDO in the reaction mixture.
Poly(octamethylene adipate-co-glyceryl adipate) were successfully produced via the N435-catalyzed co-polymerization of glycerol, adipic acid and 1,8-octanediol in bulk (Scheme 40) [280][281][282], with M n 's of up to 75,600 g/mol. The 13 C-NMR study indicated that the obtained polyesters were highly branched but had few interchain cross-links; and the degree of branching and molecular weights can be controlled by altering the reaction time and molar feed ratio of monomers [282]. In addition, due to the regio-selectivity of N435, the enzymatic polymerization gave linear polyesters at short reaction times (ď18 h) but yielded highly branched polyesters at a long reaction time (42 h). Moreover, with respect to esterifications, N435 showed 77% to 82% of the regio-selectivity towards the primary hydroxyl groups of glycerol and this was independent of the amount of glycerol in the reaction media.
The enzymatic co-polymerization of divinyl esters, glycerol and ω-fatty acids were also investigated, using lipases as biocatalysts (Scheme 42) [284,285]. Among the tested lipases, N435 showed the highest catalytic activity. The enzymatic polymerization yielded biodegradable cross-linkable polyesters with M n 's of up to 8500 g/mol. The obtained polyesters were thermally cross-linked, which resulted in transparent polymeric films with high-gloss surfaces. 31  Recently, polymeric triglyceride analogs, poly(oleic diacid-co-glycerol-co-linoleic acid)s, were prepared via the N435-catalyzed polycondensation (Scheme 44) [287]. By varying the molar feed ratio of oleic diacid, glycerol and crude linoleic acid from 1.0:1.0:1.0 to 1.0:1.0:1.33, the and dispersity of the obtained products decreased from 12,300 to 6300 g/mol, and 6.3 to 1.7, respectively, whereas the degree of tri-substituted units increased from 18% to 100%. In addition, when the molar feed ratio of oleic diacid, glycerol and crude linoleic acid was 1.0:1.0:0.67, all monomers were converted to polymers after 8 h reaction; and the and degree of tri-substituted units of the resulting copolyesters reached 9500 g/mol, and 64%, respectively. Scheme 44. N435-catalyzed synthesis of poly(oleic diacid-co-glycerol-co-linoleic acid) in bulk [287]. Scheme 42. N435-catalyzed co-polymerization of divinyl esters, glycerol and ω-fatty acids [284,285].
Recently, polymeric triglyceride analogs, poly(oleic diacid-co-glycerol-co-linoleic acid)s, were prepared via the N435-catalyzed polycondensation (Scheme 44) [287]. By varying the molar feed ratio of oleic diacid, glycerol and crude linoleic acid from 1.0:1.0:1.0 to 1.0:1.0:1.33, the M n and dispersity of the obtained products decreased from 12,300 to 6300 g/mol, and 6.3 to 1.7, respectively, whereas the degree of tri-substituted units increased from 18% to 100%. In addition, when the molar feed ratio of oleic diacid, glycerol and crude linoleic acid was 1.0:1.0:0.67, all monomers were converted to polymers after 8 h reaction; and the M n and degree of tri-substituted units of the resulting co-polyesters reached 9500 g/mol, and 64%, respectively. of oleic diacid, glycerol and crude linoleic acid from 1.0:1.0:1.0 to 1.0:1.0:1.33, the and dispersity of the obtained products decreased from 12,300 to 6300 g/mol, and 6.3 to 1.7, respectively, whereas the degree of tri-substituted units increased from 18% to 100%. In addition, when the molar feed ratio of oleic diacid, glycerol and crude linoleic acid was 1.0:1.0:0.67, all monomers were converted to polymers after 8 h reaction; and the and degree of tri-substituted units of the resulting copolyesters reached 9500 g/mol, and 64%, respectively. Scheme 44. N435-catalyzed synthesis of poly(oleic diacid-co-glycerol-co-linoleic acid) in bulk [287]. Scheme 44. N435-catalyzed synthesis of poly(oleic diacid-co-glycerol-co-linoleic acid) in bulk [287].

Sugar and Sugar Alcohol-Based Polyesters
Sugars and sugar alcohols can be used as starting materials for the production of biobased linear and branched functional polyesters which have various potential applications, for example, they can be used as coating materials, biodegradable and bioresorbable polymers, and optically active polymers [112].
It is difficult to synthesize polyesters with sugar and sugar alcohol units via conventional techniques, as tedious protection and de-protection steps are normally required, to prevent the gelation during the polymerization. However, these multiple-functional monomers can be directly polymerized via enzymatic polymerization, due to the highly regio-selectivity of the enzymes.
The lipase-catalyzed polymerization with D-sorbitol was first reported by Kobayashi et al. (Scheme 45) [288]. Sorbitol-based polyesters with M n 's of around 3000-12,000 g/mol were produced in moderate yields (around 40%-85%). Moreover, 1 H-and 13 C-NMR study indicated that the primary hydroxyl groups of D-sorbitol were exclusively esterified during the enzymatic polymerization. However, to compensate the low catalytic reactivity of N435 in the polar aprotic solvent acetonitrile, activated divinyl sebacate and high concentration of N435 (76 wt %) were used. Sugars and sugar alcohols can be used as starting materials for the production of biobased linear and branched functional polyesters which have various potential applications, for example, they can be used as coating materials, biodegradable and bioresorbable polymers, and optically active polymers [112].
It is difficult to synthesize polyesters with sugar and sugar alcohol units via conventional techniques, as tedious protection and de-protection steps are normally required, to prevent the gelation during the polymerization. However, these multiple-functional monomers can be directly polymerized via enzymatic polymerization, due to the highly regio-selectivity of the enzymes.
The lipase-catalyzed polymerization with D-sorbitol was first reported by Kobayashi et al. (Scheme 45) [288]. Sorbitol-based polyesters with 's of around 3000-12,000 g/mol were produced in moderate yields (around 40%-85%). Moreover, 1 H-and 13 C-NMR study indicated that the primary hydroxyl groups of D-sorbitol were exclusively esterified during the enzymatic polymerization. However, to compensate the low catalytic reactivity of N435 in the polar aprotic solvent acetonitrile, activated divinyl sebacate and high concentration of N435 (76 wt %) were used. Scheme 45. N435-catalyzed polymerization of D-sorbitol with divinyl sebacate [288].
Unactivated diacid monomers were also used as starting materials for the enzymatic synthesis of sorbitol-based polyesters. Gross et al. [280,281] reported the N435-catalyzed polycondensation of D-sorbitol, 1,8-octanediol and adipic acid in bulk (Scheme 46). Poly(sorbityl adipate) and poly(octamethylene adipate-co-sorbityl adipate)s were produced, with M n 's and dispersities of around 7000-20,300 g/mol, and 1.6-3.3, respectively. In addition, the molar percentage of sorbityl units in the co-polyesters can be tunable from 0% to 100%. Moreover, the NMR analysis revealed that N435 showed highly regio-selectivity (ě85%˘5%) towards the primary hydroxyl groups of D-sorbitol at 1-and 6-positions [280]. Recently, sorbitol-based, hydroxy-functional polyesters were successfully synthesized via the N435-catalyzed co-polymerization (Scheme 47) [291]. The of the resulting co-polyesters was successfully controlled at around 4000-8000 g/mol, by tuning the reaction time, enzyme concentration and reaction stoichiometry. However, only maximum 53% of the added D-sorbitol was incorporated into the final products, even though its feed ratio was quite low (≤5 mol %). Besides, the obtained polyesters displayed suitable properties for being used as solvent-borne coating resins. Scheme 47. N435-catalyzed co-polymerization of D-sorbitol, alkane-α,ω-aliphatic linear diols and diacids or diesters in bulk.
Isosorbide was enzymatically polymerized with various aliphatic diacid ethyl esters in the presence of N435 (Scheme 48), as reported by Catalani et al. [292]. The solvent-free enzymatic polymerization gave low molecular weight poly(isosorbide adipate) ( ≤ 3800 g/mol), as the hydroxyl groups of isosorbide can be condensed by N435. However, high molecular weight isosorbide polyesters with 's of up to 40,000 g/mol were produced via the enzymatic polymerization by azeotropic distillation; and significantly higher molecular weight products can be obtained by decreasing the concentration of reactants in the reaction media. Meanwhile, it was found that the suitable solvents for the enzymatic polymerization were cyclohexane, cyclohexane/benzene Scheme 46. N435-catalyzed co-polymerization of adipic acid and 1,8-octanediol with different sugar diols in bulk [280,281,290].
In the same laboratory, the enzymatic polycondensation of adipic acid and 1,8-octanediol with different sugar alcohols was investigated (Scheme 46) [290]. Sweet co-polyesters with M w 's ranging from 11,000 and 73,000 g/mol were obtained; and no correlation was observed between the reactivity of the tested sugar diols and their chain length. However, N435 showed the highest reactivity towards D-mannitol; and the co-polyester containing D-mannitol units possessed the highest degree of branching.
Recently, sorbitol-based, hydroxy-functional polyesters were successfully synthesized via the N435-catalyzed co-polymerization (Scheme 47) [291]. The M n of the resulting co-polyesters was successfully controlled at around 4000-8000 g/mol, by tuning the reaction time, enzyme concentration and reaction stoichiometry. However, only maximum 53% of the added D-sorbitol was incorporated into the final products, even though its feed ratio was quite low (ď5 mol %). Besides, the obtained polyesters displayed suitable properties for being used as solvent-borne coating resins. Recently, sorbitol-based, hydroxy-functional polyesters were successfully synthesized via the N435-catalyzed co-polymerization (Scheme 47) [291]. The of the resulting co-polyesters was successfully controlled at around 4000-8000 g/mol, by tuning the reaction time, enzyme concentration and reaction stoichiometry. However, only maximum 53% of the added D-sorbitol was incorporated into the final products, even though its feed ratio was quite low (≤5 mol %). Besides, the obtained polyesters displayed suitable properties for being used as solvent-borne coating resins. Scheme 47. N435-catalyzed co-polymerization of D-sorbitol, alkane-α,ω-aliphatic linear diols and diacids or diesters in bulk.
Isosorbide was enzymatically polymerized with various aliphatic diacid ethyl esters in the presence of N435 (Scheme 48), as reported by Catalani et al. [292]. The solvent-free enzymatic polymerization gave low molecular weight poly(isosorbide adipate) (M w ď 3800 g/mol), as the hydroxyl groups of isosorbide can be condensed by N435. However, high molecular weight isosorbide polyesters with M w 's of up to 40,000 g/mol were produced via the enzymatic polymerization by azeotropic distillation; and significantly higher molecular weight products can be obtained by decreasing the concentration of reactants in the reaction media. Meanwhile, it was found that the suitable solvents for the enzymatic polymerization were cyclohexane, cyclohexane/benzene (6:1, v/v) and cyclohexane/toluene (6:1, v/v). Furthermore, the enzymatic azeotropic polymerization in cyclohexane/toluene gave isosorbide polyesters with a higher M w when the chain length of the tested aliphatic diacid ethyl esters increased from C4 to C6. However, by further increasing the chain length from C6 to C8, C10 and 12, isosorbide polyesters with lower molecular weights were produced. (6:1, v/v) and cyclohexane/toluene (6:1, v/v). Furthermore, the enzymatic azeotropic polymerization in cyclohexane/toluene gave isosorbide polyesters with a higher when the chain length of the tested aliphatic diacid ethyl esters increased from C4 to C6. However, by further increasing the chain length from C6 to C8, C10 and 12, isosorbide polyesters with lower molecular weights were produced. Scheme 48. N435-catalyzed synthesis of isosorbide polyesters [292].
The same research group also investigated the N435-catalyzed azeotropic polycondensation of isosorbide/isomannide and diethyl adipate with different fractions of unsaturated diesters (Scheme 49) [293]. No homo-polyesters and co-polyesters containing itaconate units were obtained via the enzymatic polymerization. However, high molecular weight isosorbide/isomanide-based unsaturated co-polyesters were produced from the enzymatic azeotropic polymerization with the other tested unsaturated diesters, with 's of up to 15,900 g/mol. Moreover, Michael additions of water to C=C bonds occurred during the enzymatic polymerization; and the corresponding polymers can undergo additional reactions through hydroxyl pendant groups. Besides, the enzymatic polymerization involving isosorbide gave much higher molecular weights products, which suggested that N435 prefers isosorbide over isomannide. This is however in contract with the result reported by Boeriu et al. [294]. They investigated the N435-catalyzed polymerization of succinic acid with isomannide, isosorbide or isoidide in toluene/tert-butanol; and found that N435 showed preference for isomannide over isosorbide and over isoidide. They attributed this to the preference of N435 for the endo-hydroxyl groups, which is due to the fact that the transition state of esters with exo-hydroxyl groups does not form all the required hydrogen bonds for catalysis. Scheme 48. N435-catalyzed synthesis of isosorbide polyesters [292].
The same research group also investigated the N435-catalyzed azeotropic polycondensation of isosorbide/isomannide and diethyl adipate with different fractions of unsaturated diesters (Scheme 49) [293]. No homo-polyesters and co-polyesters containing itaconate units were obtained via the enzymatic polymerization. However, high molecular weight isosorbide/isomanide-based unsaturated co-polyesters were produced from the enzymatic azeotropic polymerization with the other tested unsaturated diesters, with M w 's of up to 15,900 g/mol. Moreover, Michael additions of water to C=C bonds occurred during the enzymatic polymerization; and the corresponding polymers can undergo additional reactions through hydroxyl pendant groups. Besides, the enzymatic polymerization involving isosorbide gave much higher molecular weights products, which suggested that N435 prefers isosorbide over isomannide. This is however in contract with the result reported by Boeriu et al. [294]. They investigated the N435-catalyzed polymerization of succinic acid with isomannide, isosorbide or isoidide in toluene/tert-butanol; and found that N435 showed preference for isomannide over isosorbide and over isoidide. They attributed this to the preference of N435 for the endo-hydroxyl groups, which is due to the fact that the transition state of esters with exo-hydroxyl groups does not form all the required hydrogen bonds for catalysis.
suggested that N435 prefers isosorbide over isomannide. This is however in contract with the result reported by Boeriu et al. [294]. They investigated the N435-catalyzed polymerization of succinic acid with isomannide, isosorbide or isoidide in toluene/tert-butanol; and found that N435 showed preference for isomannide over isosorbide and over isoidide. They attributed this to the preference of N435 for the endo-hydroxyl groups, which is due to the fact that the transition state of esters with exo-hydroxyl groups does not form all the required hydrogen bonds for catalysis. A series of Glux diacid-and Glux diol-based polyesters were synthesized via the N435-catalyzed polycondensation of diethyl sebacate and 1,4-BDO with Glux diacid/Glux diol (Scheme 50) [295]. The M w , reaction yield and intrinsic viscosity of the resulting polyesters were around 10,000 g/mol, 30%-70%, and 0.3-0.44 dL/g, respectively. In addition, the molecular weights and reaction yields of the obtained Glux diacid-based polyesters were lower than those of the synthetic Glux diol-based polyesters; and these two parameters decreased monotonically with increasing the Glux content in both Glux diacid-and Glux diol-based polyesters. Moreover, no polyester was obtained from the enzymatic polymerization of Glux diacid and 1,4-BDO. This can be explained by the bulky bicyclic structure next to the carboxylate groups, which hinders the access of this group to the active site of the enzyme CALB. Furthermore, all the synthetic polyesters possess random microstructures. A series of Glux diacid-and Glux diol-based polyesters were synthesized via the N435-catalyzed polycondensation of diethyl sebacate and 1,4-BDO with Glux diacid/Glux diol (Scheme 50) [295]. The , reaction yield and intrinsic viscosity of the resulting polyesters were around 10,000 g/mol, 30%-70%, and 0.3-0.44 dL/g, respectively. In addition, the molecular weights and reaction yields of the obtained Glux diacid-based polyesters were lower than those of the synthetic Glux diol-based polyesters; and these two parameters decreased monotonically with increasing the Glux content in both Glux diacid-and Glux diol-based polyesters. Moreover, no polyester was obtained from the enzymatic polymerization of Glux diacid and 1,4-BDO. This can be explained by the bulky bicyclic structure next to the carboxylate groups, which hinders the access of this group to the active site of the enzyme CALB. Furthermore, all the synthetic polyesters possess random microstructures. Scheme 50. N435-catalyzed synthesis of polyesters containing glucitylene or glucarate units [295].

Biobased Polyamides
At present, studies related to the enzymatic synthesis of biobased synthetic polyamides are scarcer. A few potentially biobased aliphatic polyamides, such as nylon 4,10, nylon 6,10, and nylon 8,10, can be synthesized via lipase-catalyzed polymerization. However, the molecular weights of the obtained polyamides were quite low.

Biobased Polyamides
At present, studies related to the enzymatic synthesis of biobased synthetic polyamides are scarcer. A few potentially biobased aliphatic polyamides, such as nylon 4,10, nylon 6,10, and nylon 8,10, can be synthesized via lipase-catalyzed polymerization. However, the molecular weights of the obtained polyamides were quite low.

Biobased Polyamides
At present, studies related to the enzymatic synthesis of biobased synthetic polyamides are scarcer. A few potentially biobased aliphatic polyamides, such as nylon 4,10, nylon 6,10, and nylon 8,10, can be synthesized via lipase-catalyzed polymerization. However, the molecular weights of the obtained polyamides were quite low.
In recent years, the research on FDCA-based polyesters and polyamides is booming, due to the fast development of biobased FDCA and the broad potential applications of FDCA-based polymers [16]. The FDCA-based polymers are promising sustainable aromatic polymer alternatives, and FDCA-based polymers possess similar or even better properties than their petrol-base counterparts. For example, recent studies suggested that poly(ethylene furanoate) (PEF) possesses better barrier properties compared to PET: PEF shows surprisingly large reductions in CO2 permeability (19×), O2 permeability (11×) and diffusivity (31×) [301,302].
At present, FDCA-based polyesters and polyamides are predominately synthesized via melt polycondensation at elevated temperatures of around 200 °C. However, decarboxylation of FDCA takes place at around 195 °C and other side-reactions may occur at such elevated temperatures [16,[303][304][305], which may lead to the discoloration of the resulting polymers and the formation of low molecular weight products. However, these drawbacks could be circumvented by using enzyme catalysts.
In recent years, the research on FDCA-based polyesters and polyamides is booming, due to the fast development of biobased FDCA and the broad potential applications of FDCA-based polymers [16]. The FDCA-based polymers are promising sustainable aromatic polymer alternatives, and FDCA-based polymers possess similar or even better properties than their petrol-base counterparts. For example, recent studies suggested that poly(ethylene furanoate) (PEF) possesses better barrier properties compared to PET: PEF shows surprisingly large reductions in CO 2 permeability (19ˆ), O 2 permeability (11ˆ) and diffusivity (31ˆ) [301,302].
At present, FDCA-based polyesters and polyamides are predominately synthesized via melt polycondensation at elevated temperatures of around 200˝C. However, decarboxylation of FDCA takes place at around 195˝C and other side-reactions may occur at such elevated temperatures [16,[303][304][305], which may lead to the discoloration of the resulting polymers and the formation of low molecular weight products. However, these drawbacks could be circumvented by using enzyme catalysts.
Recently, we studied the N435-catalyzed polymerization of BHMF and various diacid ethyl esters, using the two-stage, three step method (Scheme 54) [308]. BHMF-based polyesters with low molecular weights were produced, with M w 's of around 1800-2900 g/mol. The polymerization kinetic study and MALDI-ToF MS analysis revealed that ether end groups were formed during the enzymatic polymerization, which led to the low molecular weights. Furthermore, high molecular weight FDCA-based furanic-aliphatic polyamides were produced from the enzymatic polycondensation of dimethyl FDCA and 1,8-ODA, using a one-stage method or Scheme 54. N435-catalyzed polycondensation of BHMF and diacid ethyl esters via a two-stage, three step method in diphenyl ether at 80˝C [308].
FDCA-based furanic-aliphatic polyesters were successfully produced via the enzymatic polymerization of dimethyl FDCA with various aliphatic diols, using a two-stage method in diphenyl ether at 80-140˝C (Scheme 55) [309]. The obtained polyesters reached a very high M w of up to 100,000 g/mol, which is normally hard to achieve by enzymatic polymerization. For the first time we demonstrated that enzymatic polymerizations are capable of producing high molecular weight FDCA-based polyesters, which have been primarily synthesized via step-growth polymerization using organometallic catalysts at elevated temperatures around 150-280˝C. Moreover, we found that CALB prefers alkane-α,ω-aliphatic linear diols of > 3 carbons. Furthermore, the FDCA-based furanic-aliphatic polyesters possess similar crystalline and thermal properties compared to their petrol-based counterparts, semi-aromatic polyesters. Scheme 54. N435-catalyzed polycondensation of BHMF and diacid ethyl esters via a two-stage, three step method in diphenyl ether at 80 °C [308]. Scheme 55. N435-catalyzed polycondensation of dimethyl FDCA and aliphatic diol via a two-stage method in diphenyl ether [309].
Furthermore, high molecular weight FDCA-based furanic-aliphatic polyamides were produced from the enzymatic polycondensation of dimethyl FDCA and 1,8-ODA, using a one-stage method or a temperature-varied two-stage method (Scheme 56) [310]. The FDCA-based furanic-aliphatic polyamides can be used as a promising sustainable alternatives to petrol-based polyphthalamides (semi-aromatic polyamides) and be applied as thermoplastic engineering polymers and high performance materials. The enzymatic polymerization resulted in poly(octamethylene furanamide) (PA 8,F) with a very high of up to 54,000 g/mol. This is the first time that FDCA-based polyamides are successfully produced via enzymatic polymerization; and the molecular weights of the obtained PA 8,F are much higher than those produced via melt-polycondensation, the primarily synthesis approach for semi-aromatic polyamides, at elevated temperatures usually above 200 °C. Scheme 55. N435-catalyzed polycondensation of dimethyl FDCA and aliphatic diol via a two-stage method in diphenyl ether [309].
Furthermore, high molecular weight FDCA-based furanic-aliphatic polyamides were produced from the enzymatic polycondensation of dimethyl FDCA and 1,8-ODA, using a one-stage method or a temperature-varied two-stage method (Scheme 56) [310]. The FDCA-based furanic-aliphatic polyamides can be used as a promising sustainable alternatives to petrol-based polyphthalamides (semi-aromatic polyamides) and be applied as thermoplastic engineering polymers and high performance materials. The enzymatic polymerization resulted in poly(octamethylene furanamide) (PA 8,F) with a very high M w of up to 54,000 g/mol. This is the first time that FDCA-based polyamides are successfully produced via enzymatic polymerization; and the molecular weights of the obtained PA 8,F are much higher than those produced via melt-polycondensation, the primarily synthesis approach for semi-aromatic polyamides, at elevated temperatures usually above 200˝C. Moreover, the obtained PA 8,F possesses a similar T g and similar crystal structures, a comparable T d , but a lower T m , compared to its petrol-based counterpart, poly(octamethylene terephthalamide) (PA 8,T).

Conclusions and Outlook
Enzymatic polymerization is proven to be a powerful and versatile approach for the production of biobased polyesters and polyamides with different chemical compositions (aliphatic and semiaromatic polymers), varied architectures (linear, branched and hyperbranched polymers), and diverse functionalities (pendant hydroxyl groups, carbon-carbon double bonds, epoxy groups, and so on). Among the enzymes studied for biobased polyester and polyamide synthesis, CALB, especially its immobilized form N435, shows broad monomer adaptability, stable and excellent catalytic performance, and great tolerance of various conditions. Moreover, with the mild synthetic conditions, non-toxic and renewable enzyme catalysts, and sustainable starting materials, synthesis of biobased polymers via enzymatic polymerizations provides an opportunity for achieving green polymers and a future sustainable polymer industry, which will eventually play an essential role for realizing and maintaining a green and sustainable society.
However, this approach also possesses some limitations and disadvantages: (1) the atom efficiency is low when ester derivatives rather than acids are used; (2) non-ecofriendly solvents including diphenyl ether and toluene are commonly used; (3) long polymerization times are required for achieving high molecular weights; (4) high reaction temperatures at around 100-140 °C were applied for enzymatic synthesis of polymers having a high Tm and low solubility; and the catalytic reactivity of enzymes decreases significantly at such elevated temperatures; Scheme 56. N435-catalyzed polycondensation of dimethyl FDCA and 1,8-octanediamine via a one-stage method in toluene and a temperature varied two-stage method in diphenyl ether [310].

Conclusions and Outlook
Enzymatic polymerization is proven to be a powerful and versatile approach for the production of biobased polyesters and polyamides with different chemical compositions (aliphatic and semi-aromatic polymers), varied architectures (linear, branched and hyperbranched polymers), and diverse functionalities (pendant hydroxyl groups, carbon-carbon double bonds, epoxy groups, and so on). Among the enzymes studied for biobased polyester and polyamide synthesis, CALB, especially its immobilized form N435, shows broad monomer adaptability, stable and excellent catalytic performance, and great tolerance of various conditions. Moreover, with the mild synthetic conditions, non-toxic and renewable enzyme catalysts, and sustainable starting materials, synthesis of biobased polymers via enzymatic polymerizations provides an opportunity for achieving green polymers and a future sustainable polymer industry, which will eventually play an essential role for realizing and maintaining a green and sustainable society.
However, this approach also possesses some limitations and disadvantages: (1) the atom efficiency is low when ester derivatives rather than acids are used; (2) non-ecofriendly solvents including diphenyl ether and toluene are commonly used; (3) long polymerization times are required for achieving high molecular weights; (4) high reaction temperatures at around 100-140˝C were applied for enzymatic synthesis of polymers having a high T m and low solubility; and the catalytic reactivity of enzymes decreases significantly at such elevated temperatures; (5) the price of enzyme catalysts is still quite high; (6) enzymatic polymerizations involving monomers with short chain length like 1,3-propanediol, monomers with secondary hydroxyl groups such as isosorbide and 2,3-butanediol, and polyols, generally result in low molecular weight products; (7) the purify and price of biobased monomers remain a concern; (8) last but certainly not least, only limited variety of biobased monomers are currently commercially available.
Therefore, more efforts are required to address these problems. For example, acids can be used to improve the atom efficiency, green solvents such as ionic liquids and supercritical CO 2 can be employed as the reaction media, more robust and thermal stable enzymes should be developed for enzymatic polymerizations, improved and optimal processes should be explored for the production of diverse biobased monomers with high purity and low price, and so on.
Although numerous polyesters and polyamides are readily produced by using free lipases and immobilized lipases as the catalysts, the explanations for the different polymerization results are not clear yet. This could be an interest topic for the future research.
Noteworthy is that many experimental results reveal that lipase-catalyzed polymerizations involving structurally similar monomers afford polymers with different compositions and varied molecular weights. This could be attributed to the synergistic effect caused by many reasons, for example, the specificity and selectivity of lipases towards different monomers, the physical properties of the starting materials (purity, melting temperature, and miscibility and solubility in the reaction media), the physical properties of the resulting intermediates and the final products (glass transition temperature, melting temperature, crystallization ability, and miscibility and solubility in the reaction media), the enzymatic polymerization conditions, and so on. However, such synergistic effect has not been fully understood yet, which requires systematic studies in the future. Besides, it would be of great interest to employ computer simulations to study the specificity and selectivity of lipases for the monomers in the enzymatic polymerization, as well as, the enzymatic polymerization mechanism.
At present, enzymatic polymerizations have already been poised for use in commercial process to prepare polymers targeted for cosmetic and medical applications. However, polymers including biobased polymers are still predominately produced via conventional approaches. Due to the fast development of biotechnologies and enzymatic polymerization techniques, and the increased realization of the great benefits that enzymatic polymerizations and biobased monomers have to offer, there will be more highly value-added specialty biobased polymers produced commercially via biocatalytic approach in the near future. However, for the production of biobased commodity polymers, engineering plastics and high performance polymers, the commercial enzymatic process is promising but still has a long way to go, considering the high efficiency and low cost of the current pathways to the petrol-based counterparts.