Introduction Enzyme: Asubstance that acts as a catalyst in living organisms, regulating the rate at which chemical reactions proceed without itself being altered in the process. Chemical nature All enzymes were once thought to be proteins, but since the 1980s the catalytic ability of certain nucleic acids, called ribozymes (or catalytic RNAs), has been demonstrated, refuting this axiom. Because so little is yet known about the enzymatic functioning of RNA, this discussion will focus primarily on protein enzymes. A large protein enzyme molecule is composed of one or more amino acid chains called polypeptide chains. The amino acid sequence determines the characteristic folding patterns of the protein’s structure, which is essential to enzyme specificity. If the enzyme is subjected to changes, such as fluctuations in temperature or pH, the protein structure may lose its integrity (denature) and its enzymatic ability. Denaturation is sometimes, but not always, reversible. Bound to some enzymes is an additional chemical component called a cofactor, which is a direct participant in the catalytic event and thus is required for enzymatic activity. A cofactor may be either a coenzyme—an organic molecule, such as a vitamin—or an inorganic metal ion; some enzymes require both. A cofactor may be either tightly or loosely bound to the enzyme. If tightly connected, the cofactor is referred to as a prosthetic group.(1) Nomenclature An enzyme will interact with only one type of substance or group of substances, called the substrate, to catalyze a certain kind of reaction. Because of this specificity, enzymes often have been named by adding the suffix “-ase” to the substrate’s name (as in urease, which catalyzes the breakdown of urea). Not all enzymes have been named in this manner, however, and to ease the confusion surrounding enzyme nomenclature, a classification system has been developed based on the type of reaction the enzyme catalyzes. There are six principal categories -1- and their reactions: (1) oxidoreductases: which are involved in electron transfer; (2) transferases: which transfer a chemical group from one substance to another; (3) hydrolases: which cleave the substrate by uptake of a water molecule (hydrolysis); (4) lyases: which form double bonds by adding or removing a chemical group; (5) isomerases: which transfer a group within a molecule to form an isomer; -2- (6) ligases, or synthetases: which couple the formation of various chemical bonds to the breakdown of a pyrophosphate bond in adenosine triphosphate or a similar nucleotide. Mechanism Of Enzyme Action In most chemical reactions, an energy barrier exists that must be overcome for the reaction to occur. This barrier prevents complex molecules such as proteins and nucleic acids from spontaneously degrading, and so is necessary for the preservation of life. When metabolic changes are required in a cell, however, certain of these complex molecules must be broken down, and this energy barrier must be surmounted. Heat could provide the additional needed energy (called activation energy), but the rise in temperature would kill the cell. The alternative is to lower the activation energy level through the use of a catalyst. This is the role that enzymes play. Key and lock They react with the substrate to form an intermediate complex—a “transition state”—that requires less energy for the reaction to proceed. The unstable intermediate compound quickly breaks down to form reaction products, and the unchanged enzyme is free to react with other substrate molecules. Only a certain region of the enzyme, called the active site, binds to the substrate. The active site is a groove or pocket formed by the folding pattern of the -3- protein.(2) This three-dimensional structure, together with the chemical and electrical properties of the amino acids and cofactors within the active site, permits only a particular substrate to bind to the site, thus determining the enzyme’s specificity. (figure1) enzyme; active site: The active site of an enzyme is a groove or pocket that binds a specific substrate.Encyclopædia Britannica, Inc. Enzyme synthesis and activity also are influenced by genetic control and distribution in a cell. Some enzymes are not produced by certain cells, and others are formed only when required. Enzymes are not always found uniformly within a cell; often they are compartmentalized in the nucleus, on the cell membrane, or in subcellular structures. The rates of enzyme synthesis and activity are further influenced by hormones, neurosecretions, and other chemicals that affect the cell’s internal environment. 2.Induced fit model In 1958, Daniel Koshland suggested a modification to the lock and key model: since enzymes are rather flexible structures, the active site is continuously reshaped by interactions with the substrate as the substrate interacts with the enzyme. As a result, the substrate does not simply bind to a rigid active site; the amino acid side-chains that make up the active site are molded into the precise positions that enable the -4- enzyme to perform its catalytic function. In some cases, such as glycosidases, the substrate molecule also changes shape slightly as it enters the active site. The active site continues to change until the substrate is completely bound, at which point the final shape and charge distribution is determined. Induced fit may enhance the fidelity of molecular recognition in the presence of competition and noise via the conformational proofreading mechanism.(3) Cofactors Some enzymes do not need additional components to show full activity. Others require non-protein molecules called cofactors to be bound for activity. Cofactors can be either inorganic (e.g., metal ions and iron-sulfur clusters) or organic compounds (e.g., flavin and heme). These cofactors serve many purposes; for instance, metal ions can help in stabilizing nucleophilic species within the active site. Organic cofactors can be either coenzymes, which are released from the enzyme's active site during the reaction, or prosthetic groups, which are tightly bound to an enzyme. Organic prosthetic groups can be covalently bound (e.g., biotin in enzymes such as pyruvate carboxylase).(4) Coenzymes are small organic molecules that can be loosely or tightly bound to an enzyme. Coenzymes transport chemical groups from one enzyme to another. Factors Affecting Enzyme Activity Because enzymes are not consumed in the reactions they catalyze and can be used over and over again, only a very small quantity of an enzyme is needed to catalyze a reaction. A typical enzyme molecule can convert 1,000 substrate molecules per second. The rate of an enzymatic reaction increases with increased substrate concentration, reaching maximum velocity when all active sites of the enzyme molecules are engaged. The enzyme is then said to be saturated, the rate of the reaction being determined by the speed at which the active sites can convert substrate to product. Enzyme activity can be inhibited in various ways. Competitive inhibitionoccurs when molecules very similar to the substrate molecules bind to the active site and prevent -5- binding of the actual substrate. Penicillin, for example, is a competitive inhibitor that blocks the active site of an enzyme that many bacteria use to construct their cell walls. Noncompetitive inhibition occurs when an inhibitor binds to the enzyme at a location other than the active site. In some cases of noncompetitive inhibition, the inhibitor is thought to bind to the enzyme in such a way as to physically block the normal active site. In other instances, the binding of the inhibitor is believed to change the shape of the enzyme molecule, thereby deforming its active site and preventing it from reacting with its substrate. This latter type of noncompetitive inhibition is called allosteric inhibition; the place where the inhibitor binds to the enzyme is called the allosteric site. Frequently, an end-product of a metabolic pathway serves as an allosteric inhibitor on an earlier enzyme of the pathway. This inhibition of an enzyme by a product of its pathway is a form of negative feedback.(5) Allosteric control can involve stimulation of enzyme action as well as inhibition. An activator molecule can be bound to an allosteric site and induce a reaction at the active site by changing its shape to fit a substrate that could not induce the change by itself. Common activators include hormones and the products of earlier enzymatic reactions. Allosteric stimulation and inhibition allow production of energy and materials by the cell when they are needed and inhibit production when the supply is adequate. Factors affecting Enzyme Activity The activity of an Enzyme is affected by its environmental conditions. Changing these alter the rate of reaction caused by the enzyme. In nature, organisms adjust the conditions of their enzymes to produce an Optimum rate of reaction, where necessary, or they may have enzymes which are adapted to function well in extreme conditions where they live. Temperature Increasing temperature increases the Kinetic Enery that moleculespossess. In a fluid, this means that there are more random collisionsbetween molecules per unit time. -6- Since enzymes catalyse reactions by randomly colliding with Substrate molecules, increasing temperature increases the rate of reaction, forming more product. However, increasing temperature also increases the Vibrational Energythat molecules have, specifically in this case enzyme molecules, which puts strain on the bonds that hold them together. As temperature increases, more bonds, especially the weaker Hydrogenand Ionic bonds, will break as a result of this strain. Breaking bonds within the enzyme will cause the Active Site to change shape. This change in shape means that the Active Site is less Complementaryto the shape of the Substrate, so that it is less likely to catalyse the reaction. Eventually, the enzyme will become Denatured and will no longer function. As temperature increases, more enzymes' molecules' Active Sites' shapes will be less Complementary to the shape of their Substrate, and more enzymes will be Denatured. This will decrease the rate of reaction.(6) In summary, as temperature increases, initially the rate of reaction will increase, because of increased Kinetic Energy. However, the effect of bond breaking will become greater and greater, and the rate of reaction will begin to decrease. -7- The temperature at which the maximum rate of reaction occurs is called the enzyme's Optimum Temperature. This is different for different enzymes. Most enzymes in the human body have an Optimum Temperature of around 37.0 °C. pH - Acidity and Basicity pH measures the Acidity and Basicity of a solution. It is a measure of the Hydrogen Ion (H+) concentration, and therefore a good indicator of theHydroxide Ion (OH-) concentration. It ranges from pH1 to pH14. Lower pH values mean higher H+ concentrations and lower OH- concentrations. Acid solutions have pH values below 7, and Basic solutions (alkalis are bases) have pH values above 7. Deionised water is pH7, which is termed 'neutral'. H+ and OH- Ions(9) are charged and therefore interfere with Hydrogen and Ionic bonds that hold together an enzyme, since they will be attracted or repelled by the charges created by the bonds. This interference causes a change in shape of the enzyme, and importantly, its Active Site. Different enzymes have different Optimum pH values. This is the pH value at which the bonds within them are influenced by H+ and OH- Ions in such a way that the shape of their Active Site is the most Complementary to the shape of their Substrate. At the Optimum pH, the rate of reaction is at an optimum. Any change in pH above or below the Optimum will quickly cause a decrease in the rate of reaction, since more of the enzyme molecules will have Active Sites whose shapes are not (or at least are less) Complementary to the shape of their Substrate. pH Indicators -8- Small changes a permanent in pH above change to the or below enzyme, However, extreme changes in pH can since the Optimum do not cause the bonds can be reformed. cause enzymes to Denature and permanently lose their function. Enzymes in different locations have different Optimum pH values since their environmental conditions may be different. For example, the enzyme Pepsin functions best at around pH2 and is found in the stomach, which contains Hydrochloric Acid (pH2). Concentration Changing the Enzyme and Substrate concentrations affect the rate of reaction of an enzyme-catalysed reaction. Controlling these factors in a cell is one way that an organism regulates its enzyme activity and so its Metabolism. Changing the concentration of a substance only affects the rate of reaction if it is the limiting factor: that is, it the factor that is stopping a reaction from preceding at a higher rate. (15) If it is the limiting factor, increasing concentration will increase the rate of reaction up to a point, after which any increase will not affect the rate of reaction. This is because it will no -9- longer be the limiting factorand another factor will be limiting the maximum rate of reaction. As a reaction proceeds, the rate of reaction will decrease, since the Substrate will get used up. The highest rate of reaction, known as the Initial Reaction Rate is the maximum reaction rate for an enzyme in an experimental situation. Substrate Concentration Increasing Substrate Concentration increases the rate of reaction. This is because more substrate molecules will be colliding with enzyme molecules, so more product will be formed. However, after a certain concentration, any increase will have no effecton the rate of reaction, since Substrate Concentration will no longer be the limiting factor. The enzymes will effectively become saturated, and will be working at their maximum possible rate. Enzyme Concentration Increasing Enzyme Concentration will increase the rate of reaction, as more enzymes will be colliding with substrate molecules. However, this too will only have an effect up to a certain concentration, where the Enzyme Concentration is no longer the limiting factor. - 10 - Effect of Activators Some of the enzymes require certain inorganic metallic cations, like Mg2+, Mn2+, Zn2+, Ca2+, Co2+, Cu2+, Na+, K+ etc., for their optimum activity. Rarely, anions are also needed for enzyme activity, e.g. a chloride ion (CI–) for amylase. Source of enzymes Since the late 19th century scientists have been studying animal enzyme sources. Their focus was on cancerous tumors and the effect of enzymes on them. This was because cancer cells are surrounded by protein to protect them from the immune system. They studied how trypsin, chymotrypsin and pancreatin break down protein to expose the cancer cells to the immune system. Other areas of study with enzymes include heart disease, and strokeand inflammation. Fibrin, which is a protein, contributes to these diseases by causing blood clots. Protease breaks down the fibrin and can reduce inflammation. Most people don’t know that inflammation can cause a heart attack. What are the disadvantages of animal source enzymes? If you were a vegetarian you would not want to consume them. Also, animals can be exposed to antibiotics and steroids, which wouldn’t be healthy. Thirdly, they’re weakcompared to microbial enzymes. Animal enzymes are unstable at a low pH or acidic environment. Since the stomach is acidic much of the enzyme is destroyed before it can do its job. One way to get around this would be to put the enzymes in an enteric-coated tablet. This coating doesn't dissolve in acid. Thus it dissolves in the intestine, which isn't acidic. One popular brand that's enteric-coated - 11 - is Wobenzym N. They are also temperature sensitive and since we don’t have the same body temperature as the animal source this can affect the enzyme. (20) What are the advantages of animal source enzymes? The advantage is what is called the law of similar. The law of similar is the basis of homeopathy. The theory is although the source is not human your body recognizes it as similar and therefore is able to use it more effectively. The two types of plant-based enzymes are bromelain, which comes from pineapples and papain, which comes from papayas. They are quite stable in acidic pH and are not affected by temperature. One disadvantage is they are only beneficial as digestive enzymes. They can’t be used as systemic enzymes. Another is they could contain harmful substances such as phenolic compounds. Most enzyme sources come from fungi or yeast. Some consider this plant-based but fungi are actually not plants. This is because the study of fungi has historically been a branch of botany. The most popular fungus used is called aspergillus. Over half of enzymes come from fungi and yeast, over a third from bacteria. About 8% are from animal sources and 4% from plant sources What are the advantages of microbial enzymes? They are usually cheaper to produce. They are extracted from fermented fungus or bacteria. Their enzyme contents are more controllable and predictable. Manufacturers can manipulate aspergillus fungus in order to make different types of enzymes. This is done by changing the type of aspergillus that’s used. They’re the most potent enzymes and can be up to a hundred times more effective digesting proteins, carbohydrates and fats. One doesn’t have to worry about contamination with antibiotics or steroids. The pH range is broad which makes them active in stomach acid and throughout our body. Last but not least, there is a reliable supply of raw material to make microbial enzymes. Microbial Enzymes Enzymes are biocatalysts produced by living cells to bring about specific biochemical reactions generally forming parts of the metabolic processes of the cells. Enzymes are highly specific in their action on substrates and often many different enzymes are required to bring about, by concerted action, the sequence of metabolic reactions - 12 - performed by the living cell. All enzymes which have been purified are protein in nature, and may or may not possess a nonprotein prosthetic group. The practical application and industrial use of enzymes to accomplish certain reactions apart from the cell dates back many centuries and was practiced long before the nature or function of enzymes was understood. Use of barley malt for starch conversion in brewing, and of dung for bating of hides in leather making, are examples of ancient use of enzymes. It was not until nearly the turn of this century that the causative agents or enzymes responsible for bringing about such biochemical reactions became known. Then crude preparations from certain animal tissues such as pancreas and stomach mucosa, or from plant tissues such as malt and papaya fruit, were prepared which found technical applications in the textile, leather, brewing, and other industries. Once the favorable results of employing such enzyme preparations were established, a search began for better, less expensive, and more readily available sources of such enzymes. It was found that certain microorganisms produce enzymes similar in action to the amylases of malt and pancreas, or to the proteases of the pancreas and papaya fruit. This led to the development of processes for producing such microbial enzymes on a commercial scale. Dr. Jokichi Takamine (1894, 1914) was the first person to realize the technical possibility of cultivated enzymes and to introduce them to industry. He was mainly concerned with fungal enzymes, whereas Boidin and Effront (1917) in France pioneered in the production of bacterial enzymes about 20 years later. Technological progress in this field during the last decades has been so great that, for many uses, micro' Presented at Symposium, Society for Industrial Microbiology, Storrs, Connecticut, August, 1956. bial cultivated enzymes have replaced the animal or plant enzymes. For example, in textile desizing, bacterial amylase has largely replaced malt or pancreatin. At present, only a relatively small number of microbial enzymes have found commercial application, but the number is increasing, and the field will undoubtedly be much expanded in the future.(17) Enzyme Production and purification: 1.Selection of organism The most important criteria for selecting the microorganism are that the organism should produce the maximum quantities of desired enzyme in a short time while the amounts of other metabolite produced are minimal. Once the organism is selected, strain improvement for optimising the enzyme production can be done by - 13 - appropriate methods(figure2) (mutagens, UV rays). From the organism chosen, inoculum can be prepared in a liquid medium. 2.Formulation of medium The culture medium chosen should contain all the nutrients to support adequate growth of microorganisms that will ultimately result in good quantities of enzyme production. The ingredients of the medium should be readily available at low cost and are nutritionally safe. Some of the commonly used substrates for the medium are starch hydrolysate, molasses, corn steep liquor, yeast extract, whey, and soy bean meal. Some cereals (wheat) and pulses (peanut) have also been used. The pH of the medium should be kept optimal for good microbial growth and enzyme production.(22) 3.Production process Industrial production of enzymes is mostly carried out by submerged liquid conditions and to a lesser extent by solid-substrate fermentation. In submerged culture technique, the yields are more and the chances of infection are less. Hence, this is a preferred method. However, solid substrate fermentation is historically important and still in use for the production of fungal enzymes e.g. amylases, cellulases, proteases and pectinases. The medium can be sterilized by employing batch or continuous sterilization techniques. The fermentation is started by inoculating the medium. The growth conditions (pH, temperature, O2 supply, nutrient addition) are maintained at optimal levels. The froth formation can be minimised by adding antifoam agents. - 14 - The production of enzymes is mostly carried out by batch fermentation and to a lesser extent by continuous process. The bioreactor system must be maintained sterile throughout the fermentation process. The duration of fermentation is variable around 2-7 days, in most production processes. Besides the desired enzyme(s), several other metabolites are also produced. The enzyme(s) have to be recovered and purified. 4.Recovery and purification of enzymes: The desired enzyme produced may be excreted into the culture medium (extracellular enzymes) or may be present within the cells (intracellular enzymes). Depending on the requirement, the commercial enzyme may be crude or highly purified. Further, it may be in the solid or liquid form. The steps involved in downstream processing i.e. recovery and purification steps employed will depend on the nature of the enzyme and the degree of purity desired. In general, recovery of an extracellular enzyme which is present in the broth is relatively simpler compared to an intracellular enzyme. For the release of intracellular enzymes, special techniques are needed for cell disruption. The reader must invariably refer them now and learn all the details, as they form part of enzyme technology(17). Microbial cells can be broken down by physical means (sonication, high pressure, glass beads). The cell walls of bacteria can be lysed by the enzyme lysozyme. For yeasts, the enzyme β-glucanase is used. However, enzymatic methods are expensive. The recovery and purification (briefly described below) steps will be the same for both intracellular and extracellular enzymes, once the cells are disrupted and intracellular enzymes are released. The most important consideration is to minimise the loss of desired enzyme activity.(19) 5.Removal of cell debris Filtration or centrifugation can be used to remove cell debris. 6.Removal of nucleic acids Nucleic acids interfere with the recovery and purification of enzymes. - 15 - They can be precipitated and removed by adding poly-cations such as polyamines, streptomycin and polyethyleneimine. 7.Enzyme precipitation Enzymes can be precipitated by using salts (ammonium sulfate) organic solvents (isopropanol, ethanol, and acetone). Precipitation is advantageous since the precipitated enzyme can be dissolved in a minimal volume to concentrate the enzyme. 8.Liquid-liquid partition Further concentration of desired enzymes can be achieved by liquid-liquid extraction using polyethylene glycol or polyamines. 9.Separation by chromatography There are several chromatographic techniques for separation and purification of enzymes. These include ion-exchange, size exclusion, affinity, hydrophobic interaction and dye ligand chromatography .Among these, ion- exchange chromatography is the most commonly used for enzyme purification. 10.Drying and packing The concentrated form of the enzyme can be obtained by drying. This can be done by film evaporators or freeze dryers (lyophilizers). The dried enzyme can be packed and marketed. For certain enzymes, stability can be achieved by keeping them in ammonium sulfate suspensions. All the enzymes used in foods or medical treatments must be of high grade purity, and must meet the required specifications by the regulatory bodies. These enzymes should be totally free from toxic materials, harmful microorganisms and should not cause allergic reactions. Types of Culture Media: A culture media is a special medium used in microbiological laboratories to grow different kinds of microorganisms. A growth or a culture medium is composed of different nutrients that are essential for microbial growth. Since there are many types of microorganisms, each having unique properties and requiring specific nutrients for growth, there are many types based on what nutrients they contain and what function they play in the growth of microorganisms.(18) - 16 - A culture may be solid or liquid. The solid culture media is composed of a brown jelly like substance known as agar. Different nutrients and chemicals are added to it to allow the growth of different microorganisms.(19-21) A.Broth cultures One method of bacterial culture is liquid culture, in which the desired bacteria are suspended in a liquid nutrient medium, such as Luria Broth, in an upright flask. This allows a scientist to grow up large amounts of bacteria for a variety of downstream applications. Liquid cultures are ideal for preparation of an antimicrobial assay in which the experimenter inoculates liquid broth with bacteria and lets it grow overnight (they may use a shaker for uniform growth). Then they would take aliquots of the sample to test for the antimicrobial activity of a specific drug or protein (antimicrobial peptides). B.Agar plates Microbiological cultures can be grown in petri dishes of differing sizes that have a thin layer of agar-based growth medium. Once the growth medium in the petri dish is inoculated with the desired bacteria, the plates are incubated at the optimal temperature for the growing of the selected bacteria (for example, usually at 37 degrees Celsius, or the human body temperature, for cultures from humans or animals(22), or lower for environmental cultures). After the desired level of growth is achieved, agar plates can be stored upside down in a refrigerator for an extended period of time to keep bacteria for future experiments. C.Stab cultures Stab cultures are similar to agar plates, but are formed by solid agar in a test tube. Bacteria is introduced via an inoculation needle or a pipette tip being stabbed into the center of the agar. Bacteria grow in the punctured area. Stab cultures are most commonly used for short-term storage or shipment of cultures. 1.The Preservation Culture Media This is composed of all the basic nutrients required for a microbial growth and is used to preserve a specific type of microorganism, preferably bacteria or a set of different microbial entities for a long period of time. - 17 - The basic purpose of this culture is to let these microorganisms grow safely in an ensured environment that has all the important nutrients and to protect them against any environmental damage so these organisms can be used when needed. 2.The Enrichment Culture Media This is a liquid medium which allows the microorganisms to multiply and has the essential nutrients that are required for it. It is usually composed of bacteria taken from a liquid source such as pond water. The basic nutrient broth is the most commonly used. 3.Selective Culture Media This is a special type of media which allows the growth of certain microorganisms while inhibits the growth of the others. For example if we want to isolate a specific bacteria let’s say that can with stand an acidic environment from a sample of pond water and get rid of others(23), a selective media with a low pH will be taken which will allow the growth of only those organisms that can withstand acidity and will kill the others that cannot. Examples of commonly used selective media includes: PALCAM agar medium or Mac conkey agar medium. 4.Differential Culture Media This is a media that is used for differentiating between bacteria by using an identification marker for a specific type of microorganism. The selective and differential culture media are opposites to each other in a way that one inhibits the growth of other organisms(24)while allowing the growth of some while the other does not kill the others but only highlights one type. Blood agar is a common differential culture medium used to identify bacteria that causes haemolysis in blood. 5.Resuscitation Culture Media This is a special type of media which is used for growing microorganisms that are damaged and have lost the ability to produce due to certain harmful environmental factors. This culture allows the organisms to regain their metabolism by providing the nutrients that the organisms had been deprived of. For example, a type of bacteria that requires histamine for its growth is subjected to a medium lacking this essential component its growth will be inhibited. - 18 - If the same bacteria is then placed in a medium consisting of histamine it will start to grow again. In this case the media containing histamine will act as resuscitation media. An example of a commonly used resuscitation culture media is the tryptic soya agar. 6.General Purpose MediaThe general purpose media is a media that has a multiple effect, i.e. it can be used as a selective, or a resuscitation media. Figure3:deferential batch culture 7.Isolation Culture Media An isolation culture medium is a simple agar containing solid medium that allows the growth of microorganisms in the direction of the streaks. For example the bacteria will only grow on the pattern made on the solidified agar during the streak plate method. This is the most commonly used medium in microbiological labs. 8.Fermentation Media The fermentation culture media is a liquid selective media which is used to obtain a culture of a specific organism more likely yeast or a particular toxin. The fermentation media can also be differential but mostly it is selective in nature that is allowing the growth of one type while inhibiting the growth of others. Microbial culture techniques A.Indoors:allows control over illumination, temperature, nutrient level, contamination, but it expensive. B.outdoors:make it difficult to grow specific species for extended period, and it is cheap. C.Open culture:such as in uncovered ponds and tanks. D.closed culture:such as tubes, flasks, carboys, bags....etc Examples:1.Batch culture Consist of single inoculation of cells into a container of media followed by a growing for several days under suitable condition and finally harvested when growth reaching maximum denisty(figure3).(26)(27) - 19 - Advantages of batch culture 1.simple 2.allow to change species 3.remedy defects in the system rapidly Disadvantages of batch culture 1.difficulty to prevent contamination 2.require a lot of labour to harvest, clean,sterilized, refill and inoculate containers 3.efficient and quality may be inconsistent 2.Continuous culture Nutrients are supplied to the cell culture at a constant rate in order to maintain constant volume(28). they may be:A.Turbidostate:fresh media is delivered only when cell denisity reach predetermined point, fresh media is added and an equal volume of culture is removed. B.Chemostate:nutrient medium is delivered to the culture at a constant rate by a pump. Advantages of continuous culture 1.more predictable quality 2.amenable to technological control and reduce need for labour Disadvantages of continuous culture 1.high cost and complexity 2.require high control so it is feasible for relatively small proudction scales 3.Semi-continuous culture Prolongs the use of large tank cultures by partial periodic harvesting and used for large scale production. A. Fed-batch culture It is, in the broadest sense, defined as an operational technique in biotechnological processes where one or more nutrients (substrates) are fed (supplied) to the bioreactor during cultivation and in which the product(s) remain in the bioreactor until the end of - 20 - the run (figure4). An alternative description of the method is that of a culture in which "a base medium supports initial cell culture and a feed medium is added to prevent nutrient depletion". It is also a type of semi-batch culture. In some cases, all the nutrients are fed into the bioreactor. The advantage of the fed-batch culture is that one can control concentration of fed-substrate in the culture liquid at arbitrarily desired levels (in many cases, at low levels).Generally speaking, fed-batch culture is superior to conventional batch culture when controlling concentrations of a nutrient (or nutrients) affect the yield or productivity of the desired metabolite. AMYLASE Among different types of enzymes obtained from microbial sources, amylases are the most widely used in industries. In the present study, bacteria were isolated from air exposure and screened for the production of amylase. Among four bacterial isolates, one isolate produced maximum zone of starch hydrolysis. The bacterial isolate was identified as Bacillus sp. and was later used for further characterization. Maximum yield of amylase was obtained after 48hrs of incubation. The optimum pH for enzyme activity was found to be at pH 6.8 and the optimum temperature for the activity was found to be at 37 ºC. All amylases are glycoside hydrolases and act on α-1,4-glycosidic bonds.(30-39) α-Amylase: The α-amylases : (alternative names: 1,4-α-D-glucan glucanohydrolase; glycogenase) are calciummetalloenzymes. By acting at random locations along the starch chain, α-amylase breaks down long-chain carbohydrates, yielding maltotriose and maltose from amylose, or ultimately maltose, glucose and "limit dextrin" from amylopectin. Because it can act anywhere on the substrate, α-amylase tends to be faster-acting than β-amylase. In animals, it is a major digestive enzyme, and its optimum pH is 6.7–7.0. In human physiology, both the salivary and pancreatic amylases are α-amylases. The α-amylases form is also found in plants, fungi (ascomycetes and basidiomycetes) and bacteria (Bacillus) - 21 - β-Amylase: Another form of amylase, β-amylase (alternative names: 1,4-α-D-glucan maltohydrolase; glycogenase; saccharogen amylase) is also synthesized by bacteria, fungi, and plants. Working from the non-reducing end, β-amylase catalyzes the hydrolysis of the second α-1,4 glycosidic bond, cleaving off two glucose units (maltose) at a time. During the ripening of fruit, β-amylase breaks starch into maltose, resulting in the sweet flavor of ripe fruit. Both α-amylase and β-amylase are present in seeds; β-amylase is present in an inactive form prior to germination, whereas α-amylase and proteases appear once germination has begun. Many microbes also produce amylase to degrade extracellular starches. Animal tissues do not contain β-amylase, although it may be present in microorganisms contained within the digestive tract. The optimum pH for β-amylase is 4.0–5.0[8] γ-Amylase : (alternative names: Glucan 1,4-α-glucosidase; amyloglucosidase; Exo-1,4-αglucosidase; glucoamylase; lysosomal α-glucosidase; 1,4-α-D-glucan glucohydrolase) - 22 - will cleave α(1–6) glycosidic linkages, as well as the last α(1–4)glycosidic linkages at the nonreducing end of amylose and amylopectin, yielding glucose. The γ-amylase has most acidic optimum pH of all amylases because it is most active around pH 3. Isolation of Amylase Producing Microorganisms: Soil samples were collected from different environment sources. Serial dilution was made by One gram of soil sample was serially diluted in sterilized distilled water to get a concentration range from 10-1 to 10-6 and volume of 0.1 ml of each dilution was transferred aseptically to starch agar plates. The sample was spread uniformly. The plates were incubated at 37°C for 24 hrs. The bacterial isolates were further sub cultured to obtain pure culture. Pure isolates on starch agar slants were maintained at 4ºC. Screening of potent amylase producing bacteria by starch hydrolysis test: Bacterial isolates were screened for amylolytic activity by starch hydrolysis test on starch agar plate. The microbial isolates were streaked on the starch agar plate and incubated at 37°C for 48 hrs. After incubation iodine solution was flooded with dropper for 30 seconds on the starch agar plate. Presence of blue colour around the growth indicates negative result and a clear zone of hydrolysis around the growth indicates positive result. The isolates produced clear zones of hydrolysis were considered as amylase producers and were further investigated. Morphological and Biochemical Characteristics: Gram staining, motility, indole production, methyl red, Vogues Proskauer's, citrate utilization, triple sugar iron, nitrate reduction, catalase, oxidase, gelatin liquefaction, urease, hydrolysis of casein, hydrolysis of starch were carried out. - 23 - Enzyme production media: Production medium contained (g/l) Trypticase 10gm, peptone 5gm, (NH4)2SO4 3gm, K2HPO4 2gm, L-Cysteine HCl 0.5gm, MgSO4 0.2gm.10 ml of medium was taken in a 100 ml conical flask. The flasks were sterilized in autoclave at 1210 C for 15 min and after cooling the flask was inoculated with overnight grown bacterial culture. The inoculated medium was incubated at 37oC in shaker incubator for 24 hr. At the end of the fermentation period, the culture medium was centrifuged at 5000 rpm for 15 min to obtain the crude extract, which served as enzyme source.(37-40) PURIFICATION OF ENZYME: The crude enxyme was purified using organic solvent and ammonium sulphate precipitation method. Acetone method: The crude extract is treated with different concentration of acetone. In this 30% and 50% acetone was used for purification. Acetone is slowly added to the extract to precipitate out the enzyme. This is done on an ice bath and kept for 1hr under continuous stirring. The mixture is the centrifuged at 3000 rpm for 10 min. The supernatant and pellet are separated and checked for enzyme activity. Ammonium sulphate precipitation: The crude extract is treated with different concentration of Ammonium sulphate. In this 30% and 50% Ammonium sulphate was used for purification. - 24 - Ammonium sulphate is slowly added to the extract to precipitate out the enzyme. This is done on an ice bath and kept for 1hr under continuous stirring. The mixture is the centrifuged at 3000 rpm for 10mins. The supernatant and pellet are separated and checked for enzyme activity. Mechanism of amylase action on glucoside starch bonds. Functional groups of glucoamylase and alpha-amylase from Asp. awamori, alpha-amylase from Asp. oryzae and alpha- and beta-amylases from barley malt are identified. Kinetic curves of the activity dependency on pH, values of ionization heats and photooxidative inactivation draw to the conclusion that carboxyl-imidazole system enters into the active site of the enzymes. A hypothetic mechanism of hydrolysis of alpha-1,4-glucoside bond in starch molecule by alpha- and betaamylases and of alpha-1,4- and alpha-1,6-glucoside bonds by glucoamylase is given. A theory of induced correspondence of enzyme and substrate satisfactorily explains the specificity of the enzyme action and the cause of complete starch convertion into glucose under glucoamylase action and of terminal starch hydrolysis by alpha- and beta-amylases.(40-47) Enzyme activity: Enzyme activity is determined by DNS method. 0.5ml of isolated enzyme is incubating for 10 min at 370 C with 0.5 ml of substrate (ET) & 0.5 ml of substrate for (EC). After 10 min arrest the reaction by adding 1 ml of DNS to both the tube followed by 0.5 ml of enzyme to control tube only. Then kept the tubes in boiling water bath for 15 min. The solution is then dilute with 8 ml of distilled water & read the absorbance at 540 nm. - 25 - Optimization of Amylase Production Using Solid State Fermentation: Alpha-amylase [EC 3.2.1.1] cleaves the 1,4-α-D-glycosidic linkages between adjacent glucose unit inside the linear starches, glycogen, and oligosaccharides in a random manner [48]. Multifarious uses of alpha-amylases as a major starch degrading agent in food, paper, textile, and brewing industry necessitates its prolific production that can be effectively met up by solid state fermentation (SSF) [49]. Agrowastes like wheat bran, rice bran, and coconut oil bran have replaced the high cost media generally used in submerged fermentation for alpha-amylase preparation because of their simplicity, low cost, easy availability, better productivity, and lesser water output. Additionally it solves the pollution problem occurring due to their disposal in the surrounding [50]. High starch content of almost all agrowastes (60–70% by weight) can be effectively utilized as a major nutrient source by microorganisms like bacteria, fungi, and so forth, for the synthesis of inducible alpha-amylase which is under the control of catabolic repression. Plethora of evidences exists in favor of wheat bran as the best sources among all the agrosources for extracellular amylase production [51.52]. Based on the prior knowledge of primary solid state fermentation culture condition, the present study was initiated using wheat bran as a prime source of nutrient and B. amyloliquefaciens (MTCC 1270) as the producer organism at pH 7 to increase the alpha-amylase yield through media optimization.Earlier reports are also in agreement with the fact that most of the Bacillus species, namely,Bacillus licheniformis and Bacillus stearothermophilus, are the most effective producers of alpha-amylase [52-62]. Most of the amylases are metalloenzyme requiring Ca+2 for their activity, structural integrity, and stabilization [50-55]. At least three calcium binding sites have been located on barley alpha-amylase isoform that is also visible for plants, mammals, fungi, and bacteria [60.-68]. For B. amyloliquefaciens, the calcium binding site is contributed by three conserved regions of the polypeptide chain comprising residues Gly97-Ala109, Ile217-His235, and Ser314-Ser334 [65]. Depletion of calcium ion from the binding site abolishes amylase activity. Similar stabilization effect has been provided - 26 - by chloride and nitrate ions as reported by Aghajari et al. [66]. In this work major emphasishas been given in search of conditions as well as for parameters like ions and sugar alcohols whose presence in the fermentation media stimulates alpha-amylase production from SSF. Materials and Methods Microorganism Bacillus amyloliquefaciens (MTCC 1207, IMTECH, Chandigarh) was used as working strain for solid state fermentation (SSF) extraction of alpha-amylases. All the reagents are of analytical grade (SRL). 2.2. Preparation of Inoculum and Solid State Fermentation (SSF) Wheat bran was collected from local market and solid state fermentation has been carried out with 4 gm dry wheat bran in a 100 mL Erlenmeyer flask. The moisture level of the wheat bran was adjusted to 50% (w/w) with autoclaved distilled water. The contents of the flask were autoclaved prior to the solid state fermentation. 25 mL of nutrient broth was taken in a 100 mL flask and was inoculated with a loop full of Bacillus amyloliquefaciens cells from a 24-hour-old slant and kept at 37°C in a shaker. After 16 hours of growth, 1 mL inoculum (1.5–2 × 108 cfu/mL) from this broth culture was added in the WB. It was fermented for various fermentation periods (24 and 48 hours) at different temperatures (30°, 33°, 37°, and 42°C). Enzyme Extraction After 24 and 48 hours of fermentation, the fermented media containing wheat bran were mixed with 25 mL 20 mM phosphate buffer (pH = 7.0) for 30 minutes at 4°C in a rotary shaker at 150 rpm. The suspension was then centrifuged at 8000 rpm for 15 min at 4°C. The supernatant has been collected and used for amylase assay. Amylase Assay Alpha-amylase activity of the extract was measuredby DNS method [19]. In briefthe reaction mixture containing 1% soluble starch, 20 mM phosphate buffer (pH = 7), and fermented extract was taken and incubated at 37°C for 20 minutes followed by the addition of 3,5-dinitrosalicylic acid (DNS). The amount of the reducing sugar - 27 - liberated during assay was estimated by measuring color development at 540 nm by UV-VIS spectrophotometer. 1U of amylase activity is defined as the amount of enzyme that liberated micromole of maltose per minute under standard assay condition. Protein Estimation The protein content of the extract was determined following Lowry’s method [67]. 2.6. Starch Hydrolysis A 2% starch agar plate (beef extract—0.3%, soluble starch—1%, and agar—2%) has been prepared and streaked from a 24-hour-old culture of Bacillus amyloliquefaciens. The plate was grown for 48 hours in 37°C. To check the starch hydrolysis property of alpha-amylase the plate was flooded with iodine solution. Optimization of Media 4 gram of WB was supplemented with various concentrations of ions like Ca+2, , and (0.1, 0.2, and 0.4 M) from 0.5 M respective stocks of CaCl2, NaCl, and NaNO3 salt solutions for a comparative analysis regarding the yield of alpha-amylase with that of the control WB. The relative humidity was kept constant at a level of 50% (w/w) with autoclaved distilled water. The content of the flask was autoclaved and tested for solid state fermentation for 48 hours at 37°C with the addition of 1 mL inoculum (1.5–2 × 108 cfu/mL) from the broth culture. The extraction of the enzyme was performed following the same procedure as described earlier. Similar protocol of SSF has been followed for 0.5 and 1% D-inositol and D-mannitol supplementation into the WB, with proper moisture level adjusted. Control WB was autoclaved and kept for solid state fermentation under similar experimental condition without any salt and sugar supplementation with equal inoculums size as earlier. The alpha-amylase activity has been calculated according to DNS method [19]. Statistical Analysis Effect of each parameter was studied in triplicate and graphically represented as the mean ± SD () using Origin 5. - 28 - . Results Amylase Is Able to Hydrolyze Starch The starch agar plate was inoculated with B. amyloliquefaciens (MTCC 1270) and kept for 48 hours at 37°C. The plate was flooded with iodine and clear zone of starch hydrolysis has been observed (Figure 1). This ensures that this microorganism secretes amylase that is capable of starch hydrolysis . Figure 8: Starch hydrolysis performed on a 2% starch agar plate using B. amyloliquefaciens(MTCC 1270). Production of Alpha-Amylase from B. amyloliquefaciens (MTCC 1270) Using Solid State Fermentation To optimize the appropriate fermentation period for high yield alpha-amylase production, the study had been initiated with wheat bran and B. amyloliquefaciens (MTCC 1270) for 24, 48, and 72 hours. The values of specific activity of alpha-amylase were 7.25 ± 0.25 U/mg, 14.25 ± 0.24 U/mg, and 13.5 ± 0.75 U/mg, respectively, after 24, 48, and 72 hours using SSF under identical fermentation conditions (time and temperature) (Figure 2). Fermentation conducted for longer period of time was accompanied with decline in the alpha-amylase activity caused by denaturation and degradation of enzyme products. - 29 - Figure 9: α-Amylase production from solid state fermentation using B. amyloliquefaciens(MTCC 1270) and wheat bran; black column: specific activity of αamylase from SSF extract during different fermentation time periods. Influence of Temperature on Amylase Production from SSF Temperature had profound effect on the growth of the microorganism as well as on the enzyme activity. Effect of temperature on alpha-amylase production through solid state fermentation had been tested for two fermentation hours (24, 48) and at four different temperatures (30°, 33°, 37°, and 42°C). A 24-hour SSF at 37°C yielded maximum alpha-amylase production with an activity (7.25 ± 0.25 U/mg) that had been further enhanced with longer fermentation period after 48 hours at the same temperature. Although alphaamylase production was evident at all the four temperatures studied for fermentation, 37°C was the best among all to produce maximum amylase from SSF with a specific activity of 14.25 ± 0.24 U/mg This result corroborated well with optimum temperature of alpha-amylase (data not shown) that came around 40°C using standard DNS assay method [56]. After 42°C alpha-amylase activity declined due to the metabolic heat generated as an outcome of microbial growth in the solid state fermentation medium. - 30 - Figure 10: Effect of temperature on α-amylase yield after various periods of fermentation using B. amyloliquefaciens (MTCC 1270); white column: specific activity of α-amylase from 24 hours SSF extract; black column: specific activity of αamylase from 48 hours SSF extract. Effect of Ions Present in the SSF Media on Alpha-Amylase Production Effect of calcium (Ca+2) on amylase production through solid state fermentation had been checked for 48 hours fermentation at four different temperatures (30, 33, 37, and 42°C). Effect of Ca+2 at a concentration of 100 mM had been tested with a control (without any ion). Compared to control the yield of alphaamylase increased in presence of Ca+2 Among all the temperatures, 37°C solid state fermentation carried out with calcium ion gave maximum alpha-amylase activity (27 ± 1.05 U/mg) where as in absence of calcium it was about 50% less (15 ± 1.75 U/mg). This indicated the supportive role of calcium (Ca+2) in the preservation of amylase structural integrity and stability [50]. There was a gradual increase in the specific activity of amylase from 30°C to 37°C in presence of calcium (Ca+2) with a downfall of amylase activity at 42°C (9.5 ± 1.1 U/mg). - 31 - Figure 11: Effect of 0.1 mM calcium (Ca+2) on amylase production after 48 hours of SSF at 37°C temperature; dotted column: specific activity of α-amylase in absence of calcium ion from SSF extract; black column: specific activity of α-amylase in presence of calcium ion from SSF extract. Effect of chloride and nitrate ion at various concentration ranges (100, 200, and 400 mM) had been tested in order to check the effect of negative ions on the alphaamylase yield from SSF with a control (without any ion). The result was noteworthy with respect to improved amylase activity in presence of both and salts in the SSF media. Presence of 400 mM chloride () and () in the fermentation mixture improved amylase yield from 14.5 ± 0.25 U/mg to 58 ± 3 U/mg and 68 ± 0.25 U/mg, respectively, compared to control without any salt This observation can be correlated well with an insight to the alpha-amylase crystal structure derived from porcine pancreatic source at 5 Å resolutions. Chloride ion stabilized amylase structure by making electrostatic interaction with the neighboring positively charged residues like Arg 195, Lys 257, and Arg 337, which were on the other hand very close to the active site cleft of amylase. This was in congruence with the observation by Lifshitz and Levitzky, identifying one lysine residue close to the active site region that bonded with the chloride ion if present in the vicinity of the enzyme [68]. Figure 12: Effect of anions (nitrate and chloride ions) on amylase production after 48 hours of SSF, (○): specific activity of α-amylase in presence of nitrate ion from SSF extract; (●): specific activity of α-amylase in presence of chloride ion from SSF extract. 3.5. Influence of Supplementation of Sugar Alcohol on Amylase Production from SSF - 32 - Being an inducible enzyme, alpha-amylase was sensitive to catabolite repression [65]. Addition of soluble starch encouraged amylase production by B. amyloliquefaciens [69]. SSF was conducted in presence and absence of D-inositol and mannitol at 37°C for 48 hours and the alpha-amylase activity had been presented in Figure 13. The increase in inositol and mannitol concentration in the fermentation media was accompanied with the rise in amylase activity (Figure 14). 1% inositol and mannitol had maximum amylase activity of 48.5 ± 1 U/mg and 51.24 ± 1.75 U/mg, respectively, compared to control 14.5 ± 0.25 U/mg. Figure 13: Effect of sugar alcohol (D-mannitol and D-inositol) on amylase production after 48 hours of SSF; lined column: specific activity of α-amylase in presence of inositol from SSF extract; black column: specific activity of α-amylase in presence of mannitol from SSF extract. In order to elucidate the role of all the supplements in enhancing alpha-amylase activity in the fermented extract, the extract containing alpha-amylase was subjected to thermal decay at 37°C temperature for various incubation periods ranging from 0 to 60 minutes in absence and presence of ions and sugar alcohols. D-Inositol and Dmannitol have offered considerable protection against heat induced denaturation at 37°C after one hour as manifested from the retention of residual enzyme activity around 73 and 77% compared to 52% observed for amylase in extract alone in absence of any stabilizer. Similar trend of stabilization of alpha-amylase activity in presence of various salt ions (100 mM) like calcium, chloride, and nitrate has also been noticed to be subjected under thermal denaturation under similar conditions as before. All the salt ions have protected around 80% of amylase activity compared to control without salts having activity around 52% (Figure 13). - 33 - Figure 14: Percentage residual activity of amylase in absence and presence of ions and sugar alcohols. ASSAY OF AMYLASE: ENZYME Enzyme activity of crude enzyme was performed by using DNS reagent. And the enzyme activity observed for this strain was found to be 9 U/ml. Among physical parameters, pH of the growth medium plays an important role by inducing morphological changes in microbes and inenzyme secretion. The pH change observed during the growth of microbes also affected product stability in the medium. As shown in table 2 the isolate was able to grow in the pH range of 5–8, but pH 7.0 was the optimum for the growth of the cultures. Temperature also plays the significant role in the stability in enzyme activity. 35°C was found to be optimum temperature at which enzyme activity was found to be higher. Application: Fermentation Alpha and beta amylases are important in brewing beer and liquor made from sugars derived from starch. In fermentation, yeast ingest sugars and excrete alcohol. In beer and some liquors, the sugars present at the beginning of fermentation have been produced by "mashing" grains or other starch sources (such as potatoes). In traditional beer brewing, malted barley is mixed with hot water to create a "mash," which is held at a given temperature to allow the amylases in the malted grain to convert the barley's starch into sugars. Different temperatures optimize the activity of alpha or beta amylase, resulting in different mixtures of fermentable and - 34 - unfermentable sugars. In selecting mash temperature and grain-to-water ratio, a brewer can change the alcohol content, mouthfeel, aroma, and flavor of the finished beer. In some historic methods of producing alcoholic beverages, the conversion of starch to sugar starts with the brewer chewing grain to mix it with saliva.[9] This practice is no longer widely in use. Flour additive: Amylases are used in breadmaking and to break down complex sugars, such as starch (found in flour), into simple sugars. Yeastthen feeds on these simple sugars and converts it into the waste products of alcohol and CO2. This imparts flavour and causes the bread to rise. While amylases are found naturally in yeast cells, it takes time for the yeast to produce enough of these enzymes to break down significant quantities of starch in the bread. This is the reason for long fermented doughs such as sour dough. Modern breadmaking techniques have included amylases (often in the form of malted barley) into bread improver, thereby making the process faster and more practical for commercial use. Alpha amylase is often listed as an ingredient on commercially package milled flour. Bakers with long exposure to amylase-enriched flour are at risk of developing dermatitis or asthma. Molecular biology: In molecular biology, the presence of amylase can serve as an additional method of selecting for successful integration of a reporter construct in addition to antibiotic resistance. As reporter genes are flanked by homologous regions of the structural gene for amylase, successful integration will disrupt the amylase gene and prevent starch degradation, which is easily detectable through iodine staining. Medical uses: Amylase also has medical applications in the use of Pancreatic Enzyme Replacement Therapy (PERT). It is one of the components in Sollpura (Liprotamase) to help in the breakdown of carbohydrates into simple sugars. - 35 - Other uses: An inhibitor of alpha-amylase, called phaseolamin, has been tested as a potential diet aid. When used as a food additive, amylase has E number E1100, and may be derived from swine pancreas or mould mushroom. Bacilliary amylase is also used in clothing and dishwasher detergents to dissolve starches from fabrics and dishes. Factory workers who work with amylase for any of the above uses are at increased risk of occupational asthma. Five to nine percent of bakers have a positive skin test, and a fourth to a third of bakers with breathing problems are hypersensitive to amylase. Hyperamylasemia: Blood serum amylase may be measured for purposes of medical diagnosis. A higher than normal concentration may reflect one of several medical conditions, including acute inflammation of the pancreas (it may be measured concurrently with the more specific lipase), but also perforated peptic ulcer, torsion of an ovarian cyst, strangulation, ileus, mesenteric ischemia, macroamylasemia and mumps. Amylase may be measured in other body fluids, including urine and peritoneal fluid. A January 2007 study from Washington University in St. Louis suggests that saliva tests of the enzyme could be used to indicate sleep deficits, as the enzyme increases its activity in correlation with the length of time a subject has been deprived of sleep. History: In 1831, Erhard Friedrich Leuchs (1800–1837) described the hydrolysis of starch by saliva, due to the presence of an enzyme in saliva, "ptyalin", an amylase. The modern history of enzymes began in 1833, when French chemists Anselme Payen and Jean-François Persoz isolated an amylase complex from germinating barley and named it "diastase". In 1862, Alexander Jakulowitsch Danilewsky (1838–1923) separated pancreatic amylase from trypsin.[22][23] Human evolution - 36 - Carbohydrates are a food source rich in energy. Following the agricultural revolution 12,000 years ago, human diet began to rely more on plant and animal domestication in place of hunting and gathering. This shift also symbolizes the beginning of a diet composed of 49% carbohydrates as opposed to the previous 35% observed in Paleolithic humans.[citation needed] As such, starch became a staple of human diet. Large polymers such as starch are partially hydrolyzed in the mouth by the enzyme amylase before being cleaved further into sugars. Therefore, humans that contained amylase in the saliva would benefit from increased ability to digest starch more efficiently and in higher quantities. Despite the obvious benefits, early humans did not possess salivary amylase, a trend that is also seen in evolutionary relatives of the human, such as chimpanzees and bonobos, who possess either one or no copies of the gene responsible for producing salivary amylase. This gene, AMY1, originated in the pancreas. A duplication event of the AMY1 gene allowed it to evolve salivary specificity, leading to the production of amylase in the saliva. In addition the same event occurred independently in rodents, emphasizing the importance of salivary amylase in organisms that consume relatively large amounts of starch. However, not all humans possess the same number of copies of the AMY1 gene. Populations known to rely more on carbohydrates have a higher number of AMY1 copies than human populations that, by comparison, consume little starch. The number of AMY1 gene copies in humans can range from six copies in agricultural groups such as European-American and Japanese (two high starch populations) to only 2-3 copies in hunter-gatherer societies such as the Biaka, Datog, and Yakuts. The correlation that exists between starch consumption and number of AMY1 copies specific to population suggest that more AMY1 copies in high starch populations has been selected for by natural selection and considered the favorable phenotype for those individuals. Therefore, it is most likely that the benefit of an individual possessing more copies of AMY1 in a high starch population increases fitness and produces healthier, fitter offspring. This fact is especially apparent when comparing geographically close populations with different eating habits that possess a different number of copies of the AMY1 gene. Such is the case for some Asian populations that have been shown to possess few AMY1 copies relative to some agricultural population in Asia. This offers strong evidence that natural selection has acted on this gene as opposed to the possibility that the gene has spread through genetic drift.[25] - 37 - Lipase lipase is any enzyme that catalyzes the hydrolysis of fats (lipids). Lipases are a subclass of the esterases. (80) Lipases perform essential roles in the digestion, transport and processing of dietary lipids (e.g. triglycerides, fats, oils) in most, if not all, living organisms. Genes encoding lipases are even present in certain viruses. Most lipases act at a specific position on the glycerol backbone of a lipid substrate (A1, A2 or A3)(small intestine). For example, human pancreatic lipase (HPL), which is the main enzyme that breaks down dietary fats in the human digestive system, converts triglyceride substrates found in ingested oils to monoglycerides and two fatty acids. Several other types of lipase activities exist in nature, such as phospholipases and sphingomyelinases, however these are usually treated separately from "conventional" lipases. Structure and catalytic mechanism Although a diverse array of genetically distinct lipase enzymes are found in nature; and, they represent several types of protein folds and catalytic mechanisms, most of them are built on an alpha/beta hydrolase fold and employ a chymotrypsinlike hydrolysis mechanism using a catalytic triad consisting of a serine nucleophile, a histidine base, and an acid residue (usually aspartic acid).(82-86) Figure15: Structure of lipase - 38 - Production and purification of lipase enzyme 1. Isolation and characterization of bacterial strains Petrol spilled soil sample was collected from petrol bunk situated in Coimbatore, Tamilnadu, India. Serial dilution technique was used to isolate bacterial strains. Isolated bacterial strains were subjected to Gram’s staining for morphological identification and biochemical tests such as Indole production test, Citrate utilization test, Carbohydrate fermentation test, Triple sugar iron test, Oxidase test, Catalase test, Nitrate reduction test, Hydrogen sulphidetest, Methyl red and Voges–Proskauer test were performed according to Cappuccino et al. (1996).(89) Screening of lipase producing bacterial strains Isolated bacterial strains were screened for their lipolytic activity on the basis of Tributyrin Agar plate assay method (TBA). The tributyrin agar was purchased from Himedia. Tributyrin agar media along with 1.0% (v/v) olive oil were prepared and sterilized at 121 °C for 15 min, and then sterilized media were poured into petriplate. Isolated strains were streaked on the tributyrin agar plate and it was incubated at 37 °C for 24 h to observe zone. Enzyme production media Screened positive bacterial strains were cultivated in lipase producing media for enzyme production. Lipase producing media consist of 3% yeast extract, 3% sucrose, 0.1 g (g/l) CaSO4, 0.5 g/l – KH2PO4, 0.1 g/l – MgSO4.7H20, 1% olive oil and 100 ml distilled water in a 250 ml conical flask as submerged fermentation method. Inoculated flaks were incubated at 37 °C for 24–48 h (Mobarak-Qamsari et al., 2011). Optimization of lipase producing media Production media was supplemented with different carbon and nitrogen source such as sucrose, glucose, lactose, peptone, yeast extract and ammonium sulphate at different concentration (1–5%) to determine the highest yield of lipase enzyme. Microbial growth was optimized by inoculating bacteria in an autoclaved medium that had pH varying from 5 to 10 by dissolving components of the minimal medium in the - 39 - buffer of desired pH. Temperature optimization was carried out by growing bacterial strains at temperature 32–40 °C in a shaking incubator. Effect of media components on lipase activity was measured using photoelectric colorimeter at 610 nm. Similar colorimetric measurement method was carried out by Schmidt and Blum (1978). Partial purification of lipase enzyme All purification steps were performed at room temperature. From the above lipase produced media 20 ml of each bacterial strain medium was taken and the cells were separated by centrifugation at 5000 rpm for 30 min. The supernatant was collected and enzyme was concentrated using addition of 10–100% ammonium sulphate. Fractionated enzyme samples were then subjected to dialysis process for partial purification with the help of dialysis membrane. Microorganism producing lipase The bacterial strain Pseudomonas aeruginosa used in this study was isolated from a wastewater at sidibel abbes, Algeria. The isolates were identified on the basis of various morphological, physico-chemical, and biochemical characteristics. Lipolytic bacteria are typically detected and secreened through the appearance of clearing zones by using a selective medium. Which was containing Tween 80 or olive oil as the only source of carbon? The diameter ratio of clear zone and colony was measured. - 40 - Figure: Microorganisms producing lipase Effect of physical parameters on lipase production The effect of physical parameters (pH, tempera-ture and incubation period) on lipase production was carried out on production medium containing the chemical ingredients (g/l) (Peptone 10, olive oil 10, yeast extract- 5, NaCl -1, NaH2PO4 -6.08, Na2HPO4- 8.63,at pH 7.4. One ml of sterile MgSO4.7H2O stock solution (500 g/l) was added after autoclaving). 0.1% culture was inoculated into the autoclaved medium. The flasks were incubated on rotary shaker at 100 rpm, at30°C for 2 days. The culture were collected at different time intervals and centrifuged at 1000rpm for 10minat 4°C. Lipase activity was estimated by titrimetry method.(90) Effect of incubation time and biomass on lipase activity The effect of incubation time and biomass on lipase activity was determined for 12-120 h. it was noted that a high biomass was obtained at 48 h of incubation and high lipase activity was found in 72 h of incubation time around 1.2U/ml (Figure 17) Effect of pH on lipase production pH and temperature are the two important environmental factors which influences the lipase production. The pH of the production medium plays a critical - 41 - role for the optimal physiological performances of the bacterial cell and the transport of various nutrient components across the cell membrane aiming at maximizing the enzyme yields. Bacillus sp. was inoculated in the lipase production medium and incubated at different pH’s namely 5.5, 6, 6.5, 7, 7.5, 8 and 8.5. At pH 8, maximum lipase activity of 1.4 U ml-1 was observed Figure 18 Effect of Temperature lipase production A comprehensive review of all bacterial lipase.states that maximum activity of lipases at pH values higher than 7 has been observed in many cases. Bacterial lipases have a neutral or alkaline optimum pH with the exception of lipase from P. fluorescensSIK W1 that had an acidic optimum pH 4.8. For the temperature optimization process, Bacillus sp. was inoculated in lipase production medium at different temperatures namely 4, 15, 25, 35 and 45°C. The optimum temperature for lipase production was found to be 30°C showing lipase units of0.62 U ml-1. The temperature 30°C and pH 8 was found to be optimum for the lipase production by the bacterial strain. Figure 19 - 42 - Effect of carbon sources The culture environment has a dramatic influence on enzyme production especially carbon and nitrogen sources playa crucial role in enzyme induction in bacteria . The major factor for the expression of lipase activity has always been carbon, since lipases are inducible enzymes and are thus generally produced in the presence of a lipid source such as oil or any other inducer, such as triacylglycerols, fatty acids, hydrolysable esters, tweens, bile salts and glycerol. However, their production is significantly influenced by other carbon sources such as sugars, polysaccharides, whey and other complex sources. Various carbon sources namely glucose, sucrose, galactose, lactose and starch were administrated at 1% in the production medium in this study. It was noted that lactose favoured high enzyme production of 75 U ml-1. The present study is in contrast with the findings of Lakshmi who reported that the production of lipase was high in medium containing glucose supported by Banerjee who also reported that some bacteria showed higher activities when grown in medium containing glucose. (Figure 20) Effect of Nitrogen source Beside carbon source, the type of nitrogen source in the medium also influenced the lipase titers in production medium. Generally, microorganisms provide high yields of lipase when organic nitrogen sources are used, such as peptone and yeast extract, which have been used for lipase production by various Bacillus sp. and - 43 - Pseudomonads sp. It was noted that among the different nitrogen sources used, peptone was found to be the most suitable nitrogen source for Bacillus lipase production.Sirisha et al has also reported peptone as the bestnitrogen source for lipase production.reported that inorganic nitrogen sources such as ammonium chloride and ammonium dihydrogen phosphate have been also reported to be effective in some bacterial sp. (Figure 21) Dairy Industry Lipases are extensively used in the dairy industry for the hydrolysis of milk fat. Current applications include the flavour enhancement of cheeses, the acceleration of cheese ripening , the manufacturing of cheese like products, and the lipolysis of butterfat and cream. The free fatty acids generated by the action of lipases on milk fat endow many diary products, particularly soft cheeses, with their specific flavour characteristics. Thus the addition of lipases that primarily release short chain (mainly C4 and C6) fatty acids lead to the development of a sharp,tangyflavour, while the release of medium chain (C12,C14) fatty acids tend to impart a soapy taste to the product. In addition, the free fatty acids take part in simple chemical reactions, as well as being converted by the microbial population of the cheese. This initiates the synthesis of flavour ingredients such as acetoacetate, beta-keto acids, methyl ketones, flavour esters and lactones.The intensive use of lipases in cheese - 44 - making started in the U.S.A after the Second World War. It was engendered by the Food and Drug Administration's ban on the import of rennet paste from Europe because of the impurity and unsatisfactory microbiology of the product. This paste was used by the manufacturers of traditional Italian cheeses ( Provolone, Romano, Mozzarela, Parmesan) and the first lipase cocktails were introduced as a substitute to create the typical lipolyticflavour of these varieties.The traditional sources of lipases for cheese flavour enhancement are animal tissues, especially pancreatic glands(bovine and porcine) and the pre-gastric tissues of young ruminants(kid,lamb,calf). The latter are more commonly used in cheese making. The commercial pre-gastric lipases are available in the form of liquid extracts, pastes and vaccum or freeze dried powders. Each type of pre-gastric lipase gives rise to its own charecteristicflavourprofile : a buttery and slightly peppery flavour(calf) ; a sharp 'piccante' flavour (kid); a strong 'pecerino' also described as 'dirty sock' flavour(lamb).A whole range of microbial lipase preparations has been developed for the cheese manufacturing industry: Mucormeihei(Piccnate, Gist-Brocades; Palatase M, Novo Nordisk), Aspergillusniger and A.oryzae (Palatase A, Novo Nordisk; Lipase AP, Amano; Flavour AGE, Chr. Hansen) and several others. These microbial lipases are used not only for flavour enhancement and the acceleration of the ripening of specific cheeses such as blue, but in some cases they have also successfully replaced pre-gastric lipases . A range of cheeses of good quality was produced by using individual microbial lipases or mixtures of several preparations.Apart from substitution of rennet paste and flavour enhancement, lipases are widely used for imitation of cheeses made from ewe's or goat's milk. Addition of lipases to cow's milk generates a flavour rather similar to that of ewe/goat milk. This is used for producing cheeses like Feta, Manchego and Romano from cow's milk. When added to certain blue cheeses, lipase imitate the taste of Roquefort, which is normally produced from sheep's milk. Similarly, the addition of lipases to pasteurised milk leads to the development of the normal flavour of Ras or Konpanisti, which traditionally are produced from raw milk.Lipases also play a crucial role in the preparation of so-called enzyme modified cheeses (EMC). EMC is a cheese that is incubated in the presence of enzymes at elevated temparature in order to produce a concentrated flavour for use as an ingredient - 45 - in other products (dips,sauses,dressings,soups,snacks etc.). Typically the concentration of free fatty acids is ten times higher in EMC than in that of the corresponding young cheese. EMC technology is widely used in the U.S.A. Detergents Enzymes can be used in the laundry detergents and automatic dish washing machines detergents. Enzymes can reduce the environmental load of detergent products, since they save energy by enabling a lower wash temperature to be used; allow the content of other, often less desirable, chemicals in detergents to be reduced; are biodegradable, leaving no harmful residues; have no negative impact on sewage treatment processes; and, do not present a risk to aquatic life. Other enzymes are currently widely used in household cleaning products. A great deal of research is currently going into developing lipases which will work under alkaline conditions as fat stain removers. Oleochemical Industry The scope for the application of lipases in the oleochemical industry is enormous. Fats and oils are produced world wide at a level of approximately 60 million tonnes per annum and a substantial part of this(more than 2 million tonnes per annum) is utilised in high energy consuming processes such as hydrolysis, glycerolysis and alcoholysis. The conditions for steam fat splitting and conventional glycerolysis of oils involve high temparatures of 240-260 degree C and high pressures (methanolysis is currently performed under slightly milder conditions). The resulting products are often unstable as obtained and require re-distillation to remove impurities and products of degradation. In addition to this, highly unsaturated heat sensitive oils cannot be used in this process without prior hydrogenation.The saving of energy and minimisation of thermal degradation are probably the major attractions in replacing the current chemical technologies with biological ones. However, in spite of their apparent superiority, enzymic methods have not as yet attained a level of commercial exploitation commensurate with their potential. There have been several communications about relatively small scale enzymic fat - 46 - splitting processes for the production of some high value polyunsaturated fatty acids and the manufacture of soap. For instance Miyoshi Oil & Fat Co., Japan, reported the commercial use of Candida cylindracea lipase in the production of soaps. The company claimed that the enzymic method yielded a superior product and was cheaper overall than the conventional Colgate-Emery process.There are probably several reasons for the generally disappointing level of commercial applications of lipase in this sector at present. First of all, the oleochemical industry is very conservative, owing to huge capital investments involved. Therefore one cannot expect rapid changes. Secondly until recently the high cost of lipases remained prohibitive for the manufacturing of bulk products. The introduction of the new generation of cheap and very thermostable enzymes should change the economic balance in favour of lipase use. Thirdly, some concern has been expressed by chemical engineers with regard to running and controlling enzymic processes on the required scale. However the recent commercialisation of several lipase based technologies has proved their feasibility unambiguosly.The future of lipases look rather promising in the context of oleochemistry.Some fats are much more valuable than others beacuse of their structure. Less valuable fats can be converted into more useful species using blending of chemical methods but these tend to give quite random products. Lipase catalysedtransesterification of cheaper oils can be used, for example to produce cocoa butter from palm mid-fraction. Pharmaceutical Industry The vast variety of synthetic pharmaceuticals and agrochemicals containing one or more chiral centres, are stll being sold as racemates. This is despite the fact that the desired biological activity resides in one particular enantiomer. A single isomer is preferable to a racemate, but there are severe technical and/or economic problems with the production of single isomers.The usefulness of lipases in the preparation of chiral synthons is well recognised. The resolution of 2-halopropionic acids, starting materials for the synthesis of phenoxypropionate herbicides is being carried out on a 100-kg scale by Chemie Linz Co.(Austria) under a license from the Massachusetts Institute of - 47 - Technology. The process is based on the selective esterification of (S)-isomers with butanolcatalysed by porcine pancreatic lipase in anhydrous hexane. Typically ,> 99% enantiomeric excess(e.e) is obtained at 75% of the theoritical yield and the resolution is complete in several hours.Generally, the lipase mediated resolution of 2-substituted propionic acids, and especially 2aryl derivatives, have been the subject of intensive investigations. A substantial body of literature exists on the production of both (R) and (S) isomers of alpha(*sub)-phenoxypropionic acids, which are useful synthons for the preparation of enantiomerically pure herbicides and non-steroidal antiinflammatory drugs (naproxen,ibuprofen) respectively. The required optically pure derivative can be obtained directly via the (trans)esterification or hydrolysis of the corresponding ester. These resolutions have been performed on a multi-kilogramme scale by several companies world-wide.Another instance of commercial application of lipases to the resolution of racemic mixtures is the hydrolysis of epoxy alcohol esters. The highly enantioselective hydrolysis of (R,S)-glycidyl butyrate has been developed by DSM-Andeno (the Netherlands). The reaction products, (R)-glycidyl esters and (R)-glycidol, are readily converted to (R)-and (S)-glycidyltosylates, which are very attractive intermediates for the preparation of optically active beta-blockers and a wide range of other products.A similar technology has been commercialized by Sepracor Inc.(USA). This company has successfully operated a multi-kilogramme scale membrane bioreactor to produce the 2(R),2(S) methyl methoxyphenylglycidate, the key intermediate in the manufacture of the optically pure cardiovascular drug diltiazem. 2(S),3(R)methoxyphenylglycidic acid, the product of enzymic hydrolysis, was found to be unstable under the conditions of the reaction, and the resultant aldehyde inhibited the lipase activity and reduced the lifetime of the enzyme. Both problems were overcome by the introduction of a multi-phase membrane reactor where the aldehyde by-product reacted in situ with bisulphite to form a non-inhibitory, water soluble adduct, extracted into the aqueous phase.Lipases have been found useful as industrial catalysts for the resolution of racemic alcohols. Enantiomerically pure endo-2-norborn-2-ol is an important chiral intermediate in the preparation of some prostaglandins, steroids and carbocyclic nucleoside analogues. Bend Research Inc(USA) have developed a - 48 - two-step resolution process . The process involved acylation of the (R)-alcohol with butyric anhydride, mediated by Candida cylindracea lipase, followed by the hydrolysis of the (R)-ester catalysed by the same enzyme. The first resolution resulted in the enantiomerically pure (S)-alcohol (e.e> 98%) and (R)-ester(e.e-78%) which was further enriched by the back conversion to (R)alcohol(e.e> 98%). the resolution was performed on a multi-kilogramme scale in a permselective membrane bioreactor specially designed to facilitate product recovery and to minimise product inhibition.Lipases are currently being used by many pharmaceutical companies world-wide for the preparation of optically active intermediates on a kilo-gramme scale. A number of relatively small biotechnological companies, such as Enzymatix in the U.K, specialise in biotransformations and offer a whole variety of intermediates prepared via lipase mediated resolution.Regioselective modifications of polyfunctional organic compounds is yet another area of expanding lipase application. In may cases, lipases have been shown to acylate or deacylate selectively one or several hydroxyl groups of similar reactivity in carbohydrates, polyhydroxylated alkaloids and steroids.Apart from the synthesis of sugar based surfactants, lipases wer successfully applied in the regioselective modification of castanospermine. a promising drug for the treatment of AIDS.Thus lipases have become a conventional research tool in many organic chemistry laboratories. As a result they are readily incorporated into synthetic routes especially when optical purity of the final product is essential. Cosmetic Industry Although the cost of lipase catalysed esterification remains too high for the manufacturing of bulk products, the synthesis of several speciality esters has found its way in the market place. Unichem International has launched the production of isopropyl myristate, isopropyl palmitate and 2ethylhexylpalmitate for use as an emollient in personal care products such as skin and sun-tan creams, bath oils etc. Immobilised Rhizomucormeihei lipase was used as a biocatalyst in the solvent free esterification, which was driven to completion by vaccum distillation of the water produced during the reaction. - 49 - The company claims that the use of the enzyme in place of the conventional acid catalyst gives products of much higher quality, requiring minimum downstream refining. Batches of several tonnes have been successfully produced at Unichem's factory in Spain.Wax esters have similar applications in personal care products and are also being manufactured enzymically The company uses Candida cylindracea lipase in a batch bioreactor. According to the manufaturer, the overall production cost is slightly higher the that of the conventional method, but the cost is justified by the improved quality of the final product. Medical applications Possible medical applications of lipases are under consideration, for example inhibition of the human enzyme as a method of reducing fatty acid absorption is being investigated as a possible treatment for obesity. - 50 - summary Enzymes are macromolecular biological catalysts. Enzymes accelerate chemical reactions. The molecules upon which enzymes may act are called substrates and the enzyme converts the substrates into different molecules known as products.they are active in small amount, highly specific, sensitive, colloidal in nature. Almost all metabolic processes in the cell need enzyme catalysis in order to occur at rates fast enough to sustain life. Most enzymes are proteins,althoughafewarecatalyticRNAmolecules.Thelatterarecalledribozymes.Enzym es' specificity comes from their unique three-dimensional structures. Some enzymes do not need additional components to show full activity. Others require non-protein molecules called cofactors to be bound for activity. Cofactors can be either inorganic or organic compounds. Enzymes activity affecting by different factors as enzyme concentration, substrate concentration, temperature, pH, time, coenzymes concentration, presence of inhibitors. Enzymes can come from animals, plants and microbial organisms ,generally Microbes are preferred to plants and animals as sources of enzymes as they are generally cheaper to produce, their enzyme contents are more predictable and controllable, reliable supplies of raw material of constant composition are more easily arranged, and plant and animal tissues contain more potentially harmful materials than microbes, including phenolic compounds (from plants), endogenous enzyme inhibitors and proteases. Production and purification of enzymes occure in multi-steps beginning with selection of organism, formulation of medium, production process, recovery and purification of enzymes, removal of cell debris, removal of nucleic acids, enzymes precipitation, separation by chromatography and finally drying and packing. Amylases are the major group of enzymes used for starch enzyme hydrolysis, which is required prior to further fermentation for bioethanol production in biorefinery industries. This chapter discusses the characteristics, sources, production, and applications of amylases in various Industries. The main four industrially important members of the amylase family of a wide range of applications are a‐amylase, ß‐amylase, glucoamylase (GA), and pullulanase. In general, two main cultivation - 51 - strategies are applied for amylase production‐submerged fermentation (SMF) and solid‐state fermentation. Amylases are the most important industrial enzymes based on their wide range of applications in many industries. Production of stable amylases at a high temperature, acidic pH, and calcium independence was successfully achieved by using different approaches, such as production by extermophilic microorganisms, production by recombinant microorganisms, protein engineering and amino acids mutagenesis, a chemical stabilization method, a metal ion stabilization method, and an immobilization method Lipases (triacylglycerol acylhydrolase, EC 3.1.1.3) are part of the family of hydrolases that act on carboxylic ester bonds. The physiologic role of lipases is to hydrolyze triglycerides into diglycerides, monoglycerides, fatty acids, and glycerol. These enzymes are widely found throughout the animal and plant kingdoms, as well as in molds and bacteria. Of all known enzymes, lipases have attracted the most scientific attention. In addition to their natural function of hydrolyzing carboxylic ester bonds, lipases can catalyze esterification, interesterification, and transesterification reactions in nonaqueous media. This versatility makes lipases the enzymes of choice for potential applications in the food, detergent, pharmaceutical, leather, textile, cosmetic, and paper industries. The most significant industrial applications of lipases have been mainly found in the food, detergent, and pharmaceutical sectors. Limitations of the industrial use of these enzymes have mainly been owing to their high production costs, which may be overcome by molecular technologies, enabling the production of these enzymes at high levels and in a virtually purified form. - 52 - Reference: (1) Stryer L, Berg JM, Tymoczko JL (2002). Biochemistry (5th ed.). San Francisco: W.H. Freeman. ISBN 0-7167-4955-6.open access publication – free to read (2) Murphy JM, Farhan H, Eyers PA (2017). "Bio-Zombie: the rise of pseudoenzymes in biology". Biochem Soc Trans. 45: 537–544. doi:10.1042/bst20160400. (3) Murphy JM, et al. (2014). "A robust methodology to subclassify pseudokinases based on their nucleotide-binding properties". Biochemical Journal. 457 (2): 323–334. doi:10.1042/BJ20131174. PMC 5679212 Freely accessible. PMID 24107129. (4) Schomburg I, Chang A, Placzek S, Söhngen C, Rother M, Lang M, Munaretto C, Ulas S, Stelzer M, Grote A, Scheer M, Schomburg D (January 2013). "BRENDA in 2013: integrated reactions, kinetic data, enzyme function data, improved disease classification: new options and contents in BRENDA". Nucleic Acids Research. 41 (Database issue): D764–72. doi:10.1093/nar/gks1049. PMC 3531171 Freely accessible. PMID 23203881. (5) Radzicka A, Wolfenden R (January 1995). "A proficient enzyme". Science. 267 (5194): 90–931. Bibcode:1995Sci...267...90R. doi:10.1126/science.7809611. PMID 7809611. (6) Callahan BP, Miller BG (December 2007). "OMP decarboxylase—An enigma persists". Bioorganic Chemistry. 35 (6): 465–9. doi:10.1016/j.bioorg.2007.07.004. PMID 17889251. de Réaumur RA (1752). "Observations sur la digestion des oiseaux". Histoire de l'academie royale des sciences. 1752: 266, 461. (7) Williams HS (1904). A History of Science: in Five Volumes. Volume IV: Modern Development of the Chemical and Biological Sciences. Harper and Brothers. (8) Payen A, Persoz JF (1833). "Mémoire sur la diastase, les principaux produits de ses réactions et leurs applications aux arts industriels" [Memoir on diastase, the principal products of its reactions, and their applications to the industrial arts]. Annales de chimie et de physique. 2nd (in French). 53: 73–92. (9) Manchester KL (December 1995). "Louis Pasteur (1822–1895)–chance and the prepared mind". Trends in Biotechnology. 13 (12): 511–5. doi:10.1016/S01677799(00)89014-9. PMID 8595136. (10)Holmes FL (2003). "Enzymes". In Heilbron JL. The Oxford Companion to the History of Modern Science. Oxford: Oxford University Press. p. 270. - 53 - (11) The naming of enzymes by adding the suffix "-ase" to the substrate on which the enzyme acts, has been traced to French scientist Émile Duclaux (1840–1904), who intended to honor the discoverers of diastase – the first enzyme to be isolated – by introducing this practice in his book Duclaux E (1899). Traité de microbiologie: Diastases, toxines et venins [Microbiology Treatise: diastases, toxins and venoms] (in French). Paris, France: Masson and Co. See Chapter 1, especially page 9. (12) Willstätter R (1927). "Faraday lecture. Problems and methods in enzyme research". Journal of the Chemical Society (Resumed): 1359. doi:10.1039/JR9270001359. quoted in Blow D (April 2000). "So do we understand how enzymes work?" (pdf). Structure. 8 (4): R77–R81. doi:10.1016/S09692126(00)00125-8. PMID 10801479. (13) Blake CC, Koenig DF, Mair GA, North AC, Phillips DC, Sarma VR (May 1965). "Structure of hen egg-white lysozyme. A three-dimensional Fourier synthesis at 2 Ångström resolution". Nature. 206 (4986): 757–61. Bibcode:1965Natur.206..757B. doi:10.1038/206757a0. PMID 5891407. (14) Johnson LN, Petsko GA (1999). "David Phillips and the origin of structural enzymology". Trends Biochem. Sci. 24 (7): 287–9. doi:10.1016/S0968- 0004(99)01423-1. PMID 10390620.. (15) Dunaway-Mariano D (November 2008). "Enzyme function discovery". Structure. 16 (11): 1599–600. doi:10.1016/j.str.2008.10.001. PMID 19000810. (16) Petsko GA, Ringe D (2003). "Chapter 1: From sequence to structure". Protein structure and function. London: New Science. p. 27. ISBN 978-1405119221. (17) Chen LH, Kenyon GL, Curtin F, Harayama S, Bembenek ME, Hajipour G, Whitman CP (September 1992). "4-Oxalocrotonate tautomerase, an enzyme composed of 62 amino acid residues per monomer". The Journal of Biological Chemistry. 267 (25): 17716–21. PMID 1339435. (18) Smith S (December 1994). "The animal fatty acid synthase: one gene, one polypeptide, seven enzymes". FASEB Journal. 8 (15): 1248–59. PMID 8001737. (19) Suzuki H (2015). "Chapter 7: Active Site Structure". How Enzymes Work: From Structure to Function. Boca Raton, FL: CRC Press. pp. 117–140. ISBN 978-9814463-92-8. (20) Krauss G (2003). "The Regulations of Enzyme Activity". Biochemistry of Signal Transduction and Regulation (3rd ed.). Weinheim: Wiley-VCH. pp. 89–114. ISBN 9783527605767. - 54 - (21) Jaeger KE, Eggert T (August 2004). "Enantioselective biocatalysis optimized by directed evolution". Current Opinion in Biotechnology. 15 (4): 305–13. doi:10.1016/j.copbio.2004.06.007. PMID 15358000. (22) Shevelev IV, Hübscher U (May 2002). "The 3' 5' exonucleases". Nature Reviews Molecular Cell Biology. 3 (5): 364–76. doi:10.1038/nrm804. PMID 11988770. (23) Zenkin N, Yuzenkova Y, Severinov K (July 2006). "Transcript-assisted transcriptional proofreading". Science. 313 (5786): 518–20. Bibcode:2006Sci...313..518Z. doi:10.1126/science.1127422. PMID 16873663. (24) Ibba M, Soll D (2000). "Aminoacyl-tRNA synthesis". Annual Review of Biochemistry. 69: 617–50. doi:10.1146/annurev.biochem.69.1.617. PMID 10966471. (25) Rodnina MV, Wintermeyer W (2001). "Fidelity of aminoacyl-tRNA selection on the ribosome: kinetic and structural mechanisms". Annual Review of Biochemistry. 70: 415–35. doi:10.1146/annurev.biochem.70.1.415. PMID 11395413. (26) Hofmann, 8., S. Tolzer, I. Pelletier, J. Altenbuchner, K. H. van Pee, and H. J. Hecht: 1998, 'Structural investigation ofthe cofactor-free chloroperoxidases'. 1. Mol. Biol. 279,889-900. (27) Holm, L., C. Ouzounis, C. Sander, G. Tuparev, and G. Vriend: 1992, 'A database ofprotein structure families with common folding motifs'. Protein Science 1, 16911698. (28)Holm, L. and C. Sander: 1994, 'The FSSP database of structurally aligned protein fold families.'. Nucleic Acids Res. 22, 3600-3609. ( 29) A. Rameshkumar and T. Sivasudha,(2011) “Optimization of nutritional constitute for enhanced 𝛼-amylase production by solid state fermentation )technology,” International Journal of MicrobiologicalResearch,p.148,2011. (30)P. Nigam and D. Singh (1995), “Enzyme and microbial systems involvedinstarchprocessing,”EnzymeandMicrobialTechnology [31]M.Stredansky,E.Conti,L.Navarini,andC.Bertocchi(1999),“Productionofbacteriale xopolysaccharidesbysolidsubstratefermentation,”ProcessBiochemistry. [32] I.-U. Haq, H. Ashraf, J. Iqbal, and M. A. Qadeer(2003), “Production ofalphaamylasebyBacilluslicheniformisusinganeconomical medium,”BioresourceTechnology. - 55 - [33] V.H.MulimaniandG.N.P.Ramalingam (2000),“𝛼-Amylaseproduction by solid state fermentation: a new practical approach to biotechnology courses,” Biochemical Education,2000. [34] J. Shukla and R. Kar,(2006) “Potato peel as a solid state substrate for thermostable 𝛼-amylase production by thermophilic Bacillus isolates,”WorldJournalofMicrobiologyandBiotechnology [35] P. Vijayabaskar, D. Jayalakshmi, and T. Shanka (2012), “Amylase production by moderately halophilic Bacillus cereus in solid .statefermentation,”AfricanJournalofMi-CrobiologyResearch (36)Z. Baysal, F. Uyar, and C¸. Ayteki,2003n, “Solid state fermentation for production of 𝛼-amylase by a thermotolerant Bacillus subtilisfromhot- springwater,”ProcessBiochemistrypp.1665–1668,2003. [37] A. K. Mukherjee, M. Borah, and S. K. Ra ´2009 ı, “To study the influence of different components of fermentable substrates on induction of extracellular 𝛼amylase synthesis by Bacillus subtilisDM-03 in solid-state fermentation and exploration of feasibility for inclusion of 𝛼-amylase in laundry detergent formulations,” Biochemical Engineering Journal 149–156,2009. [38]H.K.Sodhi,K.Sharma,J.K.Gupta,andS.K.Soni,2005“Production ofathermostable 𝛼-amylasefromBacillussp.PS-7bysolidstate fermentation and its synergistic use in the hydrolysis of malt starchforalcoholproduction,”ProcessBiochemistry, ,2005. [39] S.K.Soni,A.Kaur,andJ.K.Gupta, 2003“Asolidstatefermentation based bacterial 𝛼-amylase and fungal glucoamylase system and its suitability for the hydrolysis of wheat starch,” Process Biochemistry 2003. [40] A. Burhan, U. Nisa, C. G ¨ okhan, C. ¨Omer, A. Ashabil, and G. Osman,2003 “Enzymatic properties of a novel thermostable, thermophilic, alkaline and chelator resistant amylase from an alkaliphilic Bacillus sp. isolate ANT-6,” Process Biochemistry, ,2003. [41] B.A.LevineandR.J.P.Williams,1982“Calciumbindingtoproteins andotherlarge biologicalanioncenters, ”inInCalciumandCell Function, W. Y. Cheung, Ed., pp. 1–38, Academic Press, New - 56 - York,NY,USA,1982. [42] C. B. Klee and T. C. Vanaman, 1982“Calmodulin,” Advances in ProteinChemistry1982. [43] A. Kadziola, J.-I. Abe, B. Svensson, and R. Haser,1994 “Crystal and molecular structure of barley 𝛼-amylase,” Journal of Molecular Biology,1994. [44] H.S.Oh,K.H.Kim,S.W.Suh,andM.U.Choi,1991“Spectroscopic andelectrophoreticstudiesonstructuralstabilityofa-amylase from Bacillus amyloliquefaciens,” Korean Biochemistry Journal, 1991. [45]N.Aghajari,G.Feller,C.Gerday,andR.Haser,2002“Structuralbasis of 𝛼amylaseactivationbychloride,”ProteinScience,vol.11,no. 2002. (46)G.L.Miller,“Useofdinitrosalisylicacidreagentfordeterminationofreducingsugar,”A nalyticalChemistry,1959. [47] O. H. Lowry, N. J. Rosenbrough, A. L. Farr, and R. J. Randall, 1951“Protein measurement with the Folin phenol reagent,” The Journalof Biological Chemistry ,1951. (48] R. Lifshitz and A. Levitzki,1993 “Identity and properties of the chloride effector binding site in hog pancreatic 𝛼-amylase,” Biochemistry,vol.15,no.9,pp.1987– 1993,1976. [49] R.RamaandS.K.Srivastav,1995“Effectofvariouscarbonsubstrate on alpha.amylase production from Bacillusspecies,” Journal of Microbial Biotechnology1995. [50] D.Gangadharan,S.Sivaramakrishnan,K.M.Nampoothiri,and A. Pandey,2006 “Solid culturing of Bacillus amyloliquefaciens for .alphaamylaseproduction,”FoodTechnologyandBiotechnology,2006 (51)D. R. Mendu, B. V. V. Ratnam, A. Purnima, and C Ayyanna,2005 “Affinity chromatography of 𝛼-amylase from Bacillus licheniformis,” EnzymeandMicrobialTechnology, 2005. (52)J.R.Mielenz,1983“Bacillusstearothermophiluscontainsaplasmidbornegenefor 𝛼amylase,”Proceeding sof the National Academy of Sciences of the United States of America,1983. [53] S. Mishra, S. B. Noronha, and G. K. Suraishkumar,2006 “Increase in enzyme productivity by induced oxidative stress in Bacillus - 57 - subtilisculturesandanalysisofitsmechanismusingmicroarray data,”ProcessBiochemistry,2005. (54] M. J. Syu and Y. H. Chen,1997 “A study on the 𝛼-amylase fermentation performed by Bacillus amyloliquefaciens,” Chemical EngineeringJournal, ,1997. [55] B. Prakash, M. Vidyasagar, M. S. Madhukumar, G. Muralikrishna, and K. Sreeramulu, 2009“Production, purification, and characterization of two extremely halotolerant, thermostable, andalkali-stable 𝛼amylasesfromChromohalobactersp.TVSP 101,”ProcessBiochemistry, ,2009. [56] L.-L.Lin,C.-C.Chyau,andW.-H.Hsu1998,“Productionandpropertiesofarawstarch-degradingamylasefromthethermophilic and alkaliphilic Bacillus sp. TS-23,” Biotechnology and Applied Biochemistry, ,1998. [57] S.D’Amico,C.Gerday,andG.Feller,2000“Structuralsimilaritiesand evolutionary relationships in chloride-dependent 𝛼-amylases,” Gene, ,2000. [58] R. Gupta, P. Gigras, H. Mohapatra, V. K. Goswami, and B. Chauhan, 2003“Microbial 𝛼-amylases: a biotechnological perspective,”ProcessBiochemistry,vol.38,no.11,pp.1599–1616,2003. [59] T. Krishnan and A. K. Chandra1983, “Purification and characterization of 𝛼amylase from Bacillus licheniformis CUMC305,” Applied and Environmental Microbiology, vol. 46, pp. 430–437, 1983. [60] A.Vengadaramana,S.Balakumar,andV.Arasaratnam2012,“Stimulation of thermal stability of𝛼-amylase from Bacillus icheniformisATCC,6346bytreatingwithcations,”CeylonJournalof Science(BiologicalSciences),vol.41,pp.35–44,2012. [61] Z.AlQodah,H.Daghstani,P.Geopel,andW.Lafi,2007“Determinationofkineticparametersof 𝛼-amylase producing gthermophile Bacillussphaericus,” AfricanJournalofBiotechnology,vol.6,no. 6,pp.699–706,2007. [62] F.A.B.A.KhanandA.A.S.A.Husaini,2006“Enhancing𝛼-amylase and cellulase in vivo enzyme expressions on sago pith residue using Bacilllus amyloliquefaciens UMAS 1002,” Biotechnology, vol.5,no.3,pp.391–403,2006. [63] A.Tonkova1991,“EffectofglucoseandcitrateonaamylaseproductioninBacilluslicheniformis,” JournalofBasicMicrobiology,vol. 31,pp.217–222,1991. - 58 - [64] Y. C. C. Young Chul Chung, T. Kobayashi, H. Kanai, T. Akiba,andT.Kudo,1995“Purificationandpropertiesofextracellular amylase from the hyperthermophilic archaeon Thermococcus profundus DT5432,” Applied and Environmental Microbiology, vol.61,no.4,pp.1502–1506,1995. [65] A. Pandey, P. Nigam, C. R. Soccol, V. T. Soccol, D. Singh, and R.Mohan,“Advancesinmicrobialamylases2000,”Biotechnologyand AppliedBiochemistry,vol.31,no.2,pp.135–152,2000. ( 66] A.Riaz,S.A.UlQader,A.Anwar,andS.Iqbal,2009“Immobilization of a thermostable A-amylase on calcium alginate beads from Bacillus subtilisKIBGEHAR,” Australian Journal of Basic and AppliedSciences,vol.3,no.3,pp.2883– .2887,2009 C. Unakal, R. I. Kallur, and B. B. Kaliwal 2012, “Produc-tion ]40[ of𝛼amylase using banana waste by Bacillus subtilisunder solidstate fermentation,” European Journal of Ex-Perimental Biology, ,2012. [67] K. Das, R. Doley, and A. K. Mukherjee,2004 “Purification and biochemical characterization of a thermostable, alkaliphilic, extracellular 𝛼-amylase from Bacillus subtilisDM-03, a strain isolatedfromthetraditionalfermentedfoodofIndia,”Biotechnology and Applied Biochemistry, , 2004. [68] A.K.Kundu,S.Das,andT.K.Gupta,1973“Influenceofcultureand nurtitionalconditionsontheproductionofamylasebythesubmergedcultureofAspergilluso ryzae,”JournalofFermentation Technology1973. (69) S. Mahmood and S. R. Rahman,2008 “Production and partial characterization of extracellular 𝛼-amylase by Trichoderma viride,” Bangladesh Journal of Microbiology, vol. 25, no. 2, pp. 99–103,2008. (70) R. A. K. Srivastava and J. N. Baruah,1986 “Culture conditions for production of thermostable amylase byBacillus stearothermophilus,” AppliedandEnvironmentalMicrobiology, ,1986 (71)Svendsen A (2000). "Lipase protein engineering". Biochim Biophys Acta. 1543 (2): 223–228. - 59 - (72)Afonso C, Tulman E, Lu Z, Oma E, Kutish G, Rock D (1999). "The Genome of Melanoplus sanguinipes Entomologists". J Virol. 73 (1): 533–52. (73)Girod A, Wobus C, Zádori Z, Ried M, Leike K, Tijssen P, Kleinschmidt J, Hallek M (2002). "The VP1 capsid protein of adeno-associated virus type 2 is carrying a phospholipase A2 domain required for virus infectivity". J Gen Virol. 83 (Pt 5): 973–8. (74)Winkler FK; D'Arcy A; W Hunziker (1990). "Structure of human pancreatic lipase". Nature. 343 (6260): 771–774. (75)Diaz, B.L.; J. P. Arm. (2003). "Phospholipase A(2)". Prostaglandins Leukot Essent Fatty Acids. 69 (2–3): 87–97. . (76)Goñi F, Alonso A (2002). "Sphingomyelinases: enzymology and membrane activity". FEBS Lett. 531 (1): 38–46. (77)Hube B, Stehr F, Bossenz M, Mazur A, Kretschmar M, Schafer W (2000). "Secreted lipases of Candida albicans: cloning, characterisation and expression analysis of a new gene family with at least ten members". Arch. Microbiol. 174 (5): 362–374. . (78)Winkler FK; D'Arcy A; W Hunziker (1990). "Structure of human boob pancreatic lipase". Nature. 343 (6260): 771–774. . (79)Schrag J, Cygler M (1997). "Lipases and alpha/beta hydrolase fold". Methods Enzymol. Methods in Enzymology. 284: 85–107. (80)Egmond, M. R.; C. J. van Bemmel (1997). "Impact of Structural Information on Understanding of Lipolytic Function". Methods Enzymol. Methods in Enzymology. 284: 119–129. (81)Withers-Martinez C; Carriere F; Verger R; Bourgeois D; C Cambillau (1996). "A pancreatic lipase with a phospholipase A1 activity: crystal structure of a chimeric pancreatic lipase-related protein 2 from guinea pig". Structure. 4 (11): 1363–74. - 60 - (82)Brady, L.; A. M. Brzozowski; Z. S. Derewenda; E. Dodson; G. Dodson; S. Tolley; J. P. Turkenburg; L. Christiansen; B. Huge-Jensen; L. Norskov; et al. (1990). "A serine protease triad forms the catalytic centre of a triacylglycerol lipase". Nature. 343 (6260): 767–70. (83)Lowe ME (1992). "The catalytic site residues and interfacial binding of human pancreatic lipase". J Biol Chem. 267 (24): 17069–73. (84) Spiegel S; Foster D; R Kolesnick (1996). "Signal transduction through lipid second messengers". Current Opinion in Cell Biology. 8 (2): 159–67. (85)Tjoelker LW; Eberhardt C; Unger J; Trong HL; Zimmerman GA; McIntyre TM; Stafforini DM; Prescott SM; PW Gray (1995). "Plasma platelet-activating factor acetylhydrolase is a secreted phospholipase A2 with a catalytic triad". J Biol Chem. 270 (43): 25481–7. (86)Gilbert B, Rouis M, Griglio S, de Lumley L, Laplaud P (2001). "Lipoprotein lipase (LPL) deficiency: a new patient homozygote for the preponderant mutation Gly188Glu in the human LPL gene and review of reported mutations: 75 % are clustered in exons 5 and 6". Ann Genet. 44 (1): 25–32. (87)Crenon I, Foglizzo E, Kerfelec B, Verine A, Pignol D, Hermoso J, Bonicel J, Chapus C (1998). "Pancreatic lipase-related protein type I: a specialized lipase or an inactive enzyme". Protein Eng. 11 (2): 135–42. (88)De Caro J, Carriere F, Barboni P, Giller T, Verger R, De Caro A (1998). "Pancreatic lipase-related protein 1 (PLRP1) is present in the pancreatic juice of several species". Biochim Biophys Acta. 1387 (1–2): 331–41. (89)Guo Z, Xu X (2005). "New opportunity for enzymatic modification of fats and oils with industrial potentials". Org Biomol Chem. 3 (14): 2615–9. Gupta R, Gupta N, Rathi P (2004). "Bacterial lipases: an overview of production, purification and biochemical properties". Appl Microbiol Biotechnol. 64 (6): 763–81. - 61 - (90)Ban K, Kaieda M, Matsumoto T, Kondo A, Fukuda H (2001). "Whole cell biocatalyst for biodiesel fuel production utilizing Rhizopus oryzae cells immobilized within biomass support particles". Biochem Eng J. 8 (1): 39–43. (91)Harding, K.G; Dennis, J.S; von Blottnitz, H; Harrison, S.T.L (2008). "A life-cycle comparison between inorganic and biological catalysis for the production of biodiesel". Journal of Cleaner Production. 16 (13): 1368–78. Bhangale, Atul S; Beers, Kathryn L; Gross, Richard A (2012). "Enzyme(92)Catalyzed Polymerization of End-Functionalized Polymers in a Microreactor". Macromolecules. 45 (17): 7000–8. (93)Kundu, Santanu; Bhangale, Atul S; Wallace, William E; Flynn, Kathleen M; Guttman, Charles M; Gross, Richard A; Beers, Kathryn L (2011). "Continuous Flow Enzyme-Catalyzed Polymerization in a Microreactor". Journal of the American Chemical Society. 133 (15): 6006– 11. (94)Anthera Pharmaceuticals - Sollpura." Anthera Pharmaceuticals - Sollpura. N.p., n.d. Web. 21 July 2015. - 62 -