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Review of Literature 2 REVIEW OF LITERATURE -...
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Review of Literature
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RREEVVIIEEWW OOFF LLIITTEERRAATTUURREE
The review of literature pertaining to the present study entitled
“Isolation and characterization of bacterial phytase and influence of
its feed supplementation in broilers” is discussed under the following
headings:
2.1 Poultry industry
2.2 Phytic acid chemistry
2.3 Enzymes in animal feed industry
2.4 Enzymology of phytase
2.5 Organic acids and their role in animal nutrition
2.6 Phytase and citric acid supplementation in poultry diet
2.1 POULTRY INDUSTRY
Livestock sector plays an important role in socio economic development
of rural households in India. In 2006, the livestock sector has grown at an
annual rate of 5.6%, which was higher than the growth of 3.3% agricultural
sector (Ali, 2007). Compared with the rest of the livestock sector, the poultry
industry in India is more scientific and well organized and progressing towards
modernization (Balakrishnan, 2002). The broiler chicken industry has now
occupied the second place in volume in the world just after pork (Yang and
Jiang, 2005). India is now the world's fourth largest egg producer and the fifth
largest producer of broilers (Saran et al., 2005). The layer industry is growing at
5 to 7% and the broiler industry at 10 to 12% per annum in India. The poultry
industry is contributing about Rs 350 billion to the national Gross Domestic
Product (GDP). In 2006, the poultry industry had the strength of 215 million
2
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layers and 1600 million broilers and by 2010 the growth rate was expected to
increase to 245 million layers and 2500 million broilers. According to the
Ministry of Food Processing Industry, in India duing 2007, the poultry industry
was estimated at over Rs 30,000 crore and is expected to grow over Rs 60,000
crore by 2010. However, the projected growth of industry depends to a great
extent on the availability of feed ingredients to meet the requirement of nearly
20 million tonnes of feed by 2010 (Sharma et al., 2006). Figure 1 presents the
projected poultry meat and egg consumption in India.
FIGURE 1
THE PROJECTED POULTRY MEAT AND EGG CONSUMPTION IN INDIA
(Mohanty and Rajendran, 2003)
Feed, is the largest cost in broiler and egg production, constituting 70 %
of the total. The main feed ingredients are maize, soy, rice bran and groundnut
cake. Maize and soy are the most widely used. Thus, the price movements of
these two feed items will have a direct effect on the prices of eggs and broilers.
Moreover, the future growth of the poultry industry will depend on the
availability and price of maize and soy. The industry has projected that demand
for maize in 2010 will be 16.65 million tonnes and foresees a major shortfall in
Millions
Million Kilograms
Poultry meat Egg
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maize production. The poultry sector consumes about 50% of the total maize
production followed by human consumption, other livestock, starch and
breweries. The situation is the same in case of soy as well (Metha et al., 2005).
2.2 PHYTIC ACID CHEMISTRY
Feeds of intensively reared poultry typically contain a high proportion of
cereals, grain legumes and oilseed meals. These feed ingredients contain
variable concentrations of phosphorus which ranges from around 19 g/kg in
extracted rice bran to less than 1g/kg in some tubers. However, approximately
two-thirds of the phosphorus is present as phytate phosphorus. Phytate is
ubiquitous in many types of plant material (Cowieson et al., 2006a). The use of
phytate phosphorus by single stomached animals has been reported to vary
from less than 10 to over 50% (Cowieson et al., 2006b). Phytic acid content of
different plant materials is summarized in Table 1.
2.2.1 Terminology related to phytic acid and phosphorus
The compound phytic acid can be commonly called as myoinositol
hexaphosphoric acid or scientifically 1, 2, 3, 4, 5, 6 hexakis (dihydrogen
phosphate) myoinositiol. In plants, phytic acid exists in its anionic form, phytate.
In mature seeds, phytic acid is found as a complex salt of calcium, magnesium
and potassium and in some cases it is bound to proteins and starches.
This complexed or chelated molecule of phytic acid is known as phytin
(Bohn et al., 2008).
The terms used for the different forms of phosphorus are as follows:
Total phosphorus is generally referred to any and all forms of phosphorus in the
diet. Available phosphorus (aP) refers to the phosphorus that is absorbed from
the diet by the animal (i.e., feed phosphorus minus phosphorus in the distal
ileum). Retained phosphorus refers to the phosphorus that stays in the body
(i.e., feed phosphorus minus excreta phosphorus).
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TABLE 1
PHYTIC ACID CONTENT IN DIFFERENT PLANT MATERIALS
Food Phytate (mg/g dry matter)
Food Phytate (mg/g dry matter)
Cereal based
French bread 0.3 - 0.4 Oat bran 12.4 - 29.6
Mixed-flour bread (70%wheat,30%rye)
0.2 - 0.7 Oat flakes 8.2 - 10.3
Mixed-flour bread (70%rye,30%wheat)
0 - 0.3 Oat porridge 7.7 - 10.6
Sourdough rye bread 0 - 0.3 Pasta 2.2 - 8.6
Wholewheat bread 4.3 - 6.8 Maize 11.5 - 14.2
Whole rye bread 2.5 - 4.8 Sorghum 5.6 - 9.8
Unleavened wheat bread
9.2 - 19.5 Rice (polished,cooked)
1.4 - 2.9
Corn bread 5.2 - 7.1 Wild rice (cooked) 16.4 - 20.1
Legume based
Chickpea 4.9 - 6.1 Navy beans (cooked)
7.4 - 10.6
Cowpea 5.8 - 10.3 Soybeans 9.9 - 14.9
Black beans 8.5 - 11.3 Tempeh 9.1 - 10.3
White beans 9.1 - 10.9 Tofu 8.2 - 9.3
Lima beans 6.2 - 9.8 Lentils (cooked) 6.5 - 9.3
Faba beans 10.1 - 13.7 Green peas (cooked)
5.7 - 7.8
Kidney beans
cooked
8.9 - 11.2 Peanuts 16.5 -19.1
Others
Sesame seeds (toasted)
43.2 - 55.1 Soy protein concentrate
12.4 - 21.7
Soy protein isolate 4.3 - 11.7 Amaranth grain 12.6 - 14.3
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FIG 2. STRUCTURE OF PHYTIC ACID
Most of the phosphorus in plant ingredients of seed origin is present in
the phytin molecule and is referred to as phytin phosphorus (PP). Any
phosphorus that is not bound to the phytin molecule is referred to as nonphytin
phosphorus (nPP). This nPP can be chemically determined by subtracting
analyzed phytin phosphorus from analyzed phosphorus. A key difference
between aP and nPP is that the term aP includes all absorbed forms of
phosphorus and will include inorganic P (Pi) and organic P (including
phytin phosphorus), whereas nPP excludes any PP available to the animal
(Angel et al.,2002).
2.2.2 Phytic acid structure
Phytic acid is the
hexaphosphoric ester of the
hexahydric cyclic alcohol
myoinositol (Kumar et al.,
2010). Myoinositol (1,2,3,4,
5,6) hexakisphosphate has six
groups of phosphates attached
to the inositol ring. Figure 2
gives the structure of phytic acid and table 2 gives the nomenclature and
structure of different myoinositol phosphate. Using the prefix “hexakis” instead
of “hexa” indicates that the phosphates are not internally connected and the
compound is consequently a polydentate ligand, which is a chelator that can
bind to more than one coordnation site of the metal atom. Each of the
phosphate groups is esterified to the inositol ring and together they can bind
upto 12 protons in total (Bohn et al., 2008). The acidity of the protons varies
from very strong acids to very weak (pKa up to 9.4) although ionic strength of
the solution and temperature influence these values (Torres et al., 2005).
Although various structural formulae for phytic acid have been proposed,
the two which have attracted the most attention are those of Neuberg and
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Anderson. The Neuberg structure implies 18 titratable hydrogen ions
whereas that of Anderson was 12. Evidences based on nuclear magnetic
resonance data and X-ray crystallography had established Anderson’s
structure (Evans et al., 1982).
TABLE 2
NOMENCLATURE AND STRUCTURE OF DIFFERENT MYOINOSITOL PHOSPHATES
Derivatives Common name Structure
Ins Myoinositol
InsP1(IP1) Myoinositol monokisphosphate
Ins(3)P1
InsP2(IP2) Myoinositol dikisphosphate
Ins(3,4)P2 Ins(3,6)P2
InsP3(IP3) Myoinositol trikisphosphate
Ins(3,4,6)P3 Ins(1,3,4)P3 Ins(1,4,5)P3
InsP4(IP4) Myoinositol tetrakisphosphate
Ins(1,3,4,6)P4 Ins(1,3,45)P4 Ins(1,4,5,6)P4
Ins(3,4,5,6)P4
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Derivatives Common name Structure
InsP5(IP5) Myoinositol pentakisphosphate
Ins(1,3,4,5,6)P5 Ins(1,2,3,4,5)P5 Ins(1,2,4,5,6)P5
Ins(1,2,3,4,6)P5
InsP6(IP6) Myoinositol hexakisphosphate
Ins(1,2,3,4,5,6)P6
2.2.3 Formation of phytic acid in plants
Normally the salts of phytic acid are found in plant seeds, animals and
soil but the acid originates from natural mineral sources containing phosphorus
or from fertilizers (Marchner, 1997). As phosphorus containing fertilizers are
applied to the soil, plant roots pick up the phosphate at a physiological pH
mainly as PO4-3 which remains as inorganic phosphorus (P) and is esterified
through the hydroxyl group to the carbon chain (C-O-P) as a single phosphate
ester or attached to another phosphate by an energy rich pyrophosphate bond.
The rate of exchange between phosphorus and organic phosphorus in the
ester and the pyrophosphate bond is very high and this leads to plant roots
incorporating phosphorus into the organic phosphorus within a few minutes but
this is released almost immediately again into the xylem (Pelig-Ba, 2009).
Hence the proportion of total phosphorus found as phytate phosphorus
increases with the dose of phosphorus supplied to the plant. When a plant
receives a higher dose of phosphorus than it requires, surplus phosphorus
seems to be stored in the form of phytic acid. Figure 3 gives the biochemical
pathway of phytic acid formation from glucose 6 phosphate.
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FIGURE 3
BIOCHEMICAL PATHWAYS IN THE FORMATION OF PHYTIC ACID FROM GLUCOSE 6 PHOSPHATE
(Raboy, 2003)
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2.2.4 Localization of phytic acid in plants and animals
Phytin is found primarily in seeds, with its location within the seed
differing among plants (Angel et al., 2002). Ninety percent of the phytin in corn
was reported to be found in the germ portion of the kernel, whereas in wheat,
barley and rice the majority of phytate was found to be accumulated in the
aleurone cells and only minor amounts in the embryo (Bohn et al., 2008).
Phytate content was found to be much higher in the bran than in the whole
grain (Guttieri et al., 2003; Steiner et al., 2007) but also within the bran fractions
differences were noticed.
In most oilseeds and grain legumes, phytin is associated with protein
and concentrated within subcellular inclusions called globoids that are
distributed throughout the kernel; however, in soybean seeds, there appeared
to be no specific location for phytin (Angel et al., 2002). Globoids are
compartmentalised inside protein storage vacuoles in the seeds. The size of
the phytate globoids was found to depend on the amount of phytate in the
grain. In wildtype wheat, globoids upto 4 micrometer in diameter have been
detected (Antoine et al., 2004), whereas a wheat mutant with lower phytic acid
had smaller globoids, organised in clusters (Joyce et al., 2005). Location of
phytin within the seed and its chemical associations with other nutrients
seemed to influence its availability (Bohn et al., 2008).
Although most phytic acid is located in the seeds, there are plants in
which it appears to be distributed throughout. Small amounts have been found
in the aerial parts of several grass species and underground parts of carrots,
potatoes and artichokes (Abernethy et al., 1973).
Presence of phytate in animal tissue is found in a lesser extent.
Grases et al. (2001) have demonstrated using gas chromotography (GC) mass
detection methodology that highest phytate accumulation was found in brain of
rats when they were fed on diets with different phytate contents.
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2.2.5 Role of phytic acid in plants and animals
The salt form, phytate, is an anhydrous storage form of phosphate
accounting for more than 80% of the total phosphorus in cereals and legumes.
Phytic acid is also a storage form of myoinositol – an important growth factor.
The lower inositol phosphates (IP1-4) and myoinositol have been recognized as
beneficial through different biological roles (Reale et al., 2007).
Phytic acid is utilized during seed germination. In seeds, the role of
phytin is as follows: 1) a phosphorus reserve, 2) an energy store, 3) a
competitor for adenosine triphosphate during rapid biosynthesis of phytin
near seed maturity when seed metabolism is inhibited and dormancy is
induced, 4) an immobilizer of divalent cations required for the control of
cellular processes and 5) a regulator of readily available seed phosphate level
(Angel et al., 2002; Raboy, 2003). Lower inositol phosphates were found to be
involved in stress responses, membrane biogenesis and intracellular signalling
(Storcksdieck et al., 2007).
In mammalian organisms, phytic acid has been implicated in starch
digestibility and blood glucose response (Lee et al., 2006), in the prevention of
dystropic calcifications in soft tissues (Grases et al., 2004), kidney stone
formation (Selvam, 2002), in the lowering of cholesterol and triglycerides
(Onomi et al., 2004) and apparently it has been tested in toothpaste as a tool
for preventing plaque formation (Vasca et al., 2002). Numerous studies in the
medical literature have reported phytate as a broad spectrum antineoplastic agent
(Vucenik and Shamsuddin, 2003).
2.2.6 Antinutritional properties of phytic acid
Due to its chemical structure, phytic acid is a very stable molecule. It
differs from other organophosphate molecules in having a high phosphate
content, which results in a high negative charge over a wide pH range and
therefore its presence in the diet has a negative impact on the bioavailability of
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divalent and trivalent mineral ions such as Zn2+, Fe2+/3+, Ca2+, Mg2+, Mn2+ and
Cu2+ (Fredlund et al., 2006). Besides, phytate has also been reported to form
complexes with proteins at both low and high pH values. These complex formations
alter the protein structure, which might result in decreased protein solubility,
enzymatic activity and proteolytic digestibility (Kumar et al., 2010). Thus, phytic acid
is an antinutritive component in plant derived food and feed.
Furthermore, phosphorus in the form of phytic acid is largely unavailable
as a nutritional factor to monogastric animals because insufficient degradation
capabilities in the gastrointestinal tract prevent the phosphorus from being
biologically available. The excess of phosphorus bound in phytic acid is then
excreted through the faeces and spread as manure into the soil. The potential
eutrophication of fresh water streams, lakes and near coastal areas can then
cause cyanobacterial blooms, hypoxia and death of aquatic animals and
production of nitrous oxide, a potential green house gas (Vats et al., 2005).
The antinutritional effect of phytic acid causes deficiency related
diseases in monogastrics which might lead to poor quality egg and meat in
case of poultry. Phytic acid is also partially attributed to the wide spreading
human nutritional deficiencies of calcium, iron and zinc in developing countries
where the staple foods are of plant origin (Manary et al., 2002).
Phytate-metal ion complexes
The presence of phytate in the diet has a negative effect on
mineral uptake (Konietzny and Greiner, 2003; Lopez et al., 2002).
Binding assays using phytic acid show the order of binding ions as
Cu2+>Zn2+>Ni2+>Co2+>Mn2+>Fe3+>Ca2+ (Vohra et al., 1965). Despite these
results, the composition of minerals in phytic acid stores does not necessarily
follow these orders of affinity. Recent findings show that phytic acid is stored
in vivo in complexes not only with these minerals, but to a much larger extent
with magnesium, calcium and potassium (Bohn et al., 2007).
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In presence of excess phytic acid, formation of soluble complexes
between phytic acid and a metal ion displaying 1:1 stoichiometries
predominates. However, when metal ions are in excess, an insoluble solid
called phytate is formed (Torres et al., 2005) (Figure 4). In human studies,
phytic acid has been reported to inhibit absorption of iron, zinc, calcium,
magnesium and manganese but surprisingly not copper (Bohn et al., 2004;
Egli et al., 2004; Phillippy, 2006). Iron and zinc uptake have both been shown
to be inhibited when the phytic acid: metal ratio was increased above
10:1 (Gharib et al., 2006; Glahn et al., 2002). Studies on the effects of phytate on
dietary manganese, copper and magnesium are limited (Lopez et al., 2002).
Removal or degradation of phytic acid would therefore increase the
bioavailability of many cations and improve nutritional value of the meal
(Bohn et al., 2008).
FIGURE 4
STRUCTURE OF PHYTATE - METAL COMPLEX
Phytate-protein interactions
Phytate forms a strong complex with some proteins and resists their
proteolysis (Kumar et al., 2010). The interaction between phytate and protein is
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largely dependent on pH (Adeola and Sands, 2003). At a pH value lower than
the isoelectric point of proteins, phosphoric acid groups of phytate bind with the
cationic group of basic amino acid and form binary protein-phytate complexes.
They are insoluble complexes that dissolve only below pH 3.5. Such complex
formations might affect the protein structures that can hamper enzymatic
activity, protein stability and protein digestibility (Kumar et al., 2010). In vitro
studies showed that the extent of phytate-protein interaction is governed by
various factors, including pH, the source and solubility of protein and dietary
levels of calcium and magnesium (Kemme et al., 1999). If the steric conditions
are satisfactory, one phytate anion can interact with two charged groups of
protein. Naturally, the protein molecule can bind more phytate anions at the
same time, depending on the number of positively charged groups and
conformational conditions (Hidvegi and Lasztity, 2002).
It was also shown that phytate-protein complexes are less likely to be
digested by proteolytic enzymes (Cowieson et al., 2006b) and even digestive
enzymes such as pepsin, trypsin, chymotrypsin, lipase and amylase are
inhibited by phytate. This inhibition might be due to the non specific nature of
phytate- protein interactions and the chelation of calcium ions, which are
essential for the activity of trypsin and alpha amylase. The reduction in the
protease activity might also be partially responsible for poor protein digestibility
(Kumar et al., 2010).
Phytate-lipid interactions
Phytate forms lipophytins (complexes with lipid and its derivatives) along
with other nutrients (Vohra and Satyanarayana, 2003). Lipid and calcium
phytate might be involved in the formation of metallic soaps in gut lumen of
poultry, which is a major restraint for energy utilization derived from lipid
sources (Leeson, 1993). Young chicks, when fed with diets supplemented with
fat and phytate, exhibited hampered phytate phosphorus utilization and a large
percentage of fat was excreted as soap fatty acids (Matyka et al., 1990).
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Phytate-carbhohydrate interactions
Phytate intake was found to reduce the blood glucose response
(Lee et al., 2006). Phytate might have formed complexes with carbohydrates of
feedstuffs thereby reducing their solubility, adversely affecting the digestibility
and absorption of glucose. Phytate might bind with starch either directly via
hydrogen bonds or indirectly via proteins associated with starch (Rickard and
Thompson, 1997). It was suggested that ternary complexes of protein, phytic
acid and carbohydrate formed subsequently might affect the digestion rate of
starch (Hidvegi and Lasztity, 2002).
It is evident that the effects of phytic acid are attributed to its ability to form
complexes with positively charged food components, such as proteins,
carbohydrates, minerals and trace elements.
2.2.7 Toxicology of phytic acid
The presence of biologically active components such as phytates and
phenolic compounds were found to have adverse effects on intrinsic properties
of proteins. Phytic acid represents a complex class of naturally occurring
organic form of phosphorus compounds that can significantly influence the
functional and nutritional properties of foods (Sabah and Murwa, 2010).
Toxicological aspects of phytic acid were extensively studied on some of the
animal systems that included human.
Impaired magnesium bioavailability due to 15 g phytic acid/kg diet was
found to accompany by an increase in hepatic thiobarbituric acid reactive
substances and protein carbonyls as well as by a moderate decline in liver
reduced glutathione levels. The liver homogenates of rats receiving the diets
with 7.5 and 15 g phytic acid/kg respectively were much more susceptible to
iron induced lipid peroxidation than those of the controls (Rimbach and Pallauf,
1999). However, phytic acid did not seem to have any scavenging effect on
superoxide radicals generated in the xanthine/xanthine oxidase reaction.
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At marginal dietary iron supply, phytic acid supplementation reduced
apparent iron absorption, thereby decreasing liver iron concentration. Neither
phytic acid nor iron had any significant effect on liver oxidant or antioxidant
status in vivo in growing rats (Rimbach and Pallauf, 1998).
Lees and Leong (1996) have reported phytic acid toxicity to neuronal
perikornia when injected into the rat hippocampus. Its potency as a toxin was
approximately equal to that of the excitotoxin quinolinate. It was concluded by
their study that abnormal metabolism of phytic acid might possibly contribute to
neuronal death in neurodegenerative diseases. Carcinogenecity of phytic acid
has been studied and Hiasa et al. (1992) have shown necrosis and calcification
of renal papillae in Fischer 344 rats when treated with phytic acid. The rate of
colonic cancer could arise from many fibre rich foods which might contain high
phytate (Vucenik and Shamsuddin, 2003).
2.3 ENZYMES IN ANIMAL FEED INDUSTRY
Consistent increase in the price of feed ingredients has been a major
constraint in most of the developing countries. As a result, cheaper and
nonconventional feed ingredients have to be used which contain higher
percentage of nonstarch polysaccharides (soluble and insoluble/crude fibre)
along with starch (Khattak et al., 2006). In addition, consumer awareness and
new legislation require that any increase in animal production cannot be
achieved via growth promoting drugs or other chemical substances.
Consumers and industrialists are looking more closely than ever before into
how compound animal feeds are produced, how the animals are reared, the
current feeding practices and the end result of the systems of animal
husbandry to the environment (Godfrey and West, 1996). Among all, the role of
feed and nutrition for livestock production has gained attention as it can affect
the animal directly which in turn can affect the human health and the
environment (Sapkota et al., 2007).
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2.3.1 Different enzymes used in feed
The major types of enzymes used in animal feeds are categorized by
their substrate specificity. All enzyme preparations recommended for use to
improve dietary nutrient utilization in animals are found to be hydrolases
(Ferket and Santos, 2006). Commercial enzyme products are typically a blend
of several different enzymes that are effective on a wide variety of substrates
that comprise the feed. The enzymes with proven efficacies for animal
husbandry include xylanase, arabinoxylanase, β-glucanase, cellulase, phytase
(Choct and Kocher, 2000), proteases (Khattak et al., 2006) and phospholipase
(Santos et al., 2004).
For most of the enzymatic processes, microbial enzymes are preferred,
primarily because they are easier and cheaper to obtain. Microorganisms
secrete a wide variety of proteolytic enzymes. These enzymes are of
central importance and are among the most important hydrolytic enzymes
(Haq and Mukhtar, 2006). The use of enzymes impart less chemical
load on the environment, higher efficiency and the ability to dilute multiple
downstream transformation attempts while maintaining product yield and
recovery (Chandel et al., 2008).
The first commercial success was the addition of β-glucanase into
barley based feed diets. Barley contains β-glucan, which causes high viscosity
in the chicken gut. The net effect of enzyme usage in feed was reported to be
increased animal weight gain with the same amount of barley resulting in
increased feed conversion ratio. Later enzymes were also tested in wheat
based diets. Silva and Smithard (2002) studied the effect of xylanase on rye
based diets and observed that the reduction in small intestinal viscosity by the
enzyme improved nutrient digestion. Xylanases are nowadays routinely used in
feed formulations (Ferket and Santos, 2006).
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Another type of important feed enzyme is phytase. It is a
phosphoesterase which liberates phosphate from phytic acid which is a
common compound in plant based feed materials. The net effect is reduced
phosphorus in faeces resulting in reduced environmental pollution. The use of
phytase reduces the need to add phosphorus to the feed diet. Supplementation
of microbial phytase was observed to reduce the need for mineral
supplementation by increasing the availability of cations (phosphorus, calcium,
zinc and copper) bound to phytic acid (Odetallah, 2000).
The action of cellulase is complex because cellulose is generally
associated with other polymers, such as lignin and pentosans. Recently,
protease on corn soybean meal based diets has received considerable
attention. Supplementation of poultry diets with enzyme mixtures that include
proteases and amylases have produced significant improvements in growth
performance (Greenwood et al., 2002; Burrows et al., 2002).
Usually a feed enzyme preparation is a multienzyme cocktail containing
glucanases, xylanases, proteinases and amylases (Ferket and Santos, 2006).
They are normally incorporated into the grains before pelletization and the
feed briefly reaches processing temperatures of 85 - 90°C. Therefore the feed
enzymes need to be thermo tolerant (Rao et al., 2009).
2.4 ENZYMOLOGY OF PHYTASE
Lott et al. (2000) have estimated that nearly 35 million metric tons of
phytic acid, containing 9.9 million metric tons of phosphate, is combined
with about 12.5 and 3.9 million metric tons of potassium and magnesium
respectively, to form each year over 51 million metric tons of phytate. The
amount of phosphorus in this phytate was found to be equal to nearly 65% of
the elemental phosphorus sold worldwide for use in mineral fertilizers. Dry
cereal grains account for 69% of the total crop seed/fruit production but account
for 77% of the total phytic acid stored each year.
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Decrease in phytic acid was found to be very advantageous, due to its
influence on nutrition and therefore interest has grown to reduce its
antinutritional effects (Abdelrahaman et al., 2005). Also the mineral binding
capacity was found to decrease when the phosphate groups were removed
and this might reduce the adverse effects of phytate on mineral bioavailability
(Kim et al., 2008).
It is estimated that 10 kg of dicalcium phosphate can be replaced by
250 g of phytase enzyme (Gulati et al., 2007). In India, the use of phytase in
monogastric diets was estimated to be approximately 500 tons/year as reported
by Compound Livestock Feed Manufacturers Association (CLFMA, 2007).
But the phytase market in China was reported to be 5500 tons/year (Xu, 2006).
In biological system, hydrolysis of phytic acid to myoinositol and
inorganic phosphate is an important reaction for energy metabolism, metabolic
regulation and signal transduction pathways. The reaction was primarily
catalysed by phytases (myoinositol hexakisphosphate phosphohydrolase).
They are histidine acid phosphatases (HAPs), a subclass of phosphatases,
which catalyze the hydrolysis of phosphate moieties from phytic acid, thereby,
resulting in the loss of ability of phytic acid to chelate metal ions (Vats and
Banerjee, 2004).
2.4.1 Classification of phytase
The International Union of Pure and Applied Chemistry and the
International Union of Biochemistry and Molecular Biology (IUPAC-IUBMB)
have recognized three classes of phytase enzymes, 3-phytases, 5-phytases
and 6-phytases, which initiate the dephosphorylation of phytic acid at different
positions on the inositol ring and produce different isomers of the lower inositol
phosphates (Bohn et al., 2008).
Within each class of phytase, structural differences can be found and not
all enzymes within a certain class hydrolyze phosphate from phytic acid
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through the same mechanism. All phytases have pronounced stereo specificity
and a strong preference for equatorial phosphate groups over axial groups
(Lei and Porres, 2003). Figure 5 shows the end products of phytate hydrolysis
mediated by phytase enzyme from different origins.
The largest group of phytases belong to the 3-phytases (EC 3.1.3.8),
which in general are found in fungi and bacteria and initiate the hydrolysis of
phytate at the third phosphate group (Sajidan et al., 2004). Structurally,
most of the 3-phytases show homology to betapropeller phosphatase (BPP) or
histidine acid phosphatases (HAP). BPPs are tightly bound to three calcium
ions and two phosphate groups before hydrolysis can occur. The end
product has been suggested to be inositol triphosphate either Ins(1,3,5)P3 or
Ins(2,4,6)P3 (Kerovuo et al., 2000; Shin et al., 2001), but Oh et al. (2006)
reported Ins(2,4,6)P3 to be the sole end product, confirming the equatorial
preference of most phytases.
FIGURE 5
THE END PRODUCTS RESULTING FROM PHYTATE HYDROLYSIS MEDIATED BY DIFFERENT PHYTASES
Bacillus phytases
Fungal phytases
Plant phytases
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HAPs can initiate hydrolysis of phytic acid on either the C3 or the C6
position of the inositol ring and produce myoinositol monophosphate (in
particular Ins(2)P due to its axial position) as the final product (Mullaney
and Ullah, 2003; Greiner and Carlsson, 2006; Oh et al., 2006). Most bacterial,
fungal and plant phytases belong to the HAPs. Within this structural
classification, there are two phytase subgroups: some show broad
substrate specificity but low specific activity for phytic acid, whereas others
have narrow substrate specificities but high specific activity for phytic acid
(Bohn et al., 2008).
6-phytases (EC 3.1.3.26) initiate the hydrolysis of phytate at the sixth
phosphate group (Greiner et al., 1993; Kaay and Haastert, 1995). Several
structurally different phytases namely, the purple acid phosphatase (PAP), the
ADP phosphoglycerate phosphatase (related to EC 3.1.3.28) and an HAP-class
are found in this group (Bohn et al., 2008). Purple acid phosphatase is found as
a homodimeric glycoprotein in mainly plant species, with a Fe(III)-Zn(II) active
site (Dionisio et al., 2007).
The 3-phytases do not always completely dephosphorylate IP6, whereas
the 6-phytases do (Angel et al., 2002). According to the conserved domain
database (CDD) of the National Center for Biotechnologyl Information (NCBI),
the conserved domains in acid phosphatases, phytases and purple acid
phosphatases are designated as pfam00328, pfam02333 and pfam02227
respectively. 5-phytases (EC 3.1.3.72) from Medicago sativa, Phaseolus
vulgaris, and Pisum sativum which were found to initiate phytate hydrolysis at
the fifth phosphate group (Rao et al., 2009).
2.4.2 Occurrence of phytase
Natural degradation of phytic acid was observed to be almost
impossible and chemical hydrolysis in the laboratory was found to be very slow
(Turner et al., 2002). However, the enzyme phytase is found wide spread in
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27
nature (including animals, plants and microbes) which can rapidly breakdown
phytate (Mullaney and Ullah, 2003).
Plant and animal phytase
Phytase occurs widely in the plant kingdom. Phytase has been isolated
and characterized from cereals such as triticale, wheat, maize, barley and rice
and from beans such as navy beans, mung beans, dwarf beans and California
small white beans. Phytase activity has also been detected in white mustard,
potato, radish, lettuce, spinach, grass and lily pollen (Dvorakova, 1998).
Different phytases were identified in negligible quantities in the mucosal
extracts of small intestine of rats, chickens, humans, rabbits and guinea pigs
(Marounek et al., 2003).
Microbial phytase
Researches have shown that microbial phytases are most promising
for biotechnological applications (Vohra and Satyanarayana, 2003). Although
phytases from several species of bacteria, yeast and fungi have been
characterized and commercial production was mostly focused on the soil
fungus Aspergillus. However, due to some properties such as substrate
specificity, resistance to proteolysis and catalytic efficiency bacterial phytases
have proved to be real alternative to the fungal enzymes (Konietzny and
Greiner, 2004).
Phytases have been detected in various bacteria, such as
Pseudomonas sp. (Richardson and Hadobas, 1997), Bacillus sp. (Kerovuo
et al., 1998; Choi et al., 2001), Raoultella sp. (Greiner et al., 1997; Sajidan
et al., 2004), Escherichia coli (Greiner et al., 1993), Citrobacter braakii
(Kim et al., 2003), Enterobacter (Yoon et al., 1996), Lac. Sanfranciscensis
(Angelis et al., 2003) and anaerobic rumen bacteria, particularly in
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28
S. ruminantium, M. elsdenii, Prevotella sp., M.multiacidus (Yanke et al., 1998)
and M. jalaludinii (Lan et al., 2002a).
Generally, the phytases produced by fungi are extracellular, whereas the
enzymes from bacteria are mostly cell associated. The only bacteria showing
extracellular phytase activity are those of the genera Bacillus (Kim et al., 1998;
Choi et al., 2001) and Enterobacter (Yoon et al., 1996). The phytases of E. coli
have been reported to be periplasmatic enzymes (Greiner et al., 1993) and
phytase activity in S. ruminantium and M. multiacidus were found to be
associated with the outer membrane (D’Silva et al., 2000).
2.4.4 Current and potential applications of phytase
In animal feed
Phytase has been mainly, if not solely, used as a feed supplement in
diets largely for swine and poultry and to some extent for fish. Numerous
laboratory experiments and field trials have shown that 500 to 1000 units of
phytase can replace approximately 1 g inorganic phosphorus supplementation
and reduce total phosphorus excretion by 30 - 50% (Kemme et al., 1997;
Lei et al., 1993a; Liu et al., 1997; Yi et al., 1996a). The benefits of phytase
are two fold: saving the expensive and nonrenewable inorganic phosphorus
resource by reducing the need for its inclusion in animal diets and
protecting the environment from pollution of excessive manure phosphorus
runoff. Supplemental organic acids such as citric acid or lactic acid were
found to enhance phytase efficacy (Han et al., 1998; Jongbloed et al., 2000;
Maenz et al., 1999).
In human nutrition
Processing and manufacturing of human food is also a possible field of
application of phytase. No phytase product for a relevant food application is
reported to be on the market till now. Research in this field focuses on better
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29
mineral absorption or technical improvement of food processing (Haefner et al.,
2005). Some food processing methods are shown to reduce or remove
considerable amounts of phytate in legumes (Awada et al., 2005; Soetan
and Oyewole, 2009) but use of phytase could reduce the phytic acid content in
food products more efficiently. Phytase was reported to fully degrade phytic
acid during the manufacture of roller dried complementary foods based on
flours from rice, wheat, maize, oat, sorghum and a wheat soy flour blend
(Hurrell et al., 2003). Haros et al. (2001) investigated the possible use of
phytase in the process of bread making. The main achievement of this use was
the shortened fermentation period without affecting the bread dough pH. An
increase in bread volume and an improvement in crumb texture were also
observed.
In the synthesis of lower inositol
Lower phosphoric esters of myoinositol (mono, bis, tris, and
tetrakisphosphates) play a crucial role in transmembrane signaling processes
and in calcium mobilization from intracellular store in animal as well as in plant
tissues (Dasgupta et al., 1996; Krystofova et al., 1994). The use of phytase has
been shown to be very effective in producing different inositol phosphate
species. Phytase isolated from A. niger was shown to efficiently hydrolyze IP6
to all lower phosphorylated derivatives from myoinositol pentakisphosphate
(IP5) to myoinositol dikisphosphate (IP2) depending on the amount of the
enzyme (Dvorakova et al., 2000).
2.5 ORGANIC ACIDS AND THEIR ROLE IN ANIMAL NUTRITION
Besides the nutritional value, high quality feed also has a positive effect
on the health status of animals. The most efficient way to keep compound feed
at a high hygienic status is the use of organic acids. Acids with an antifungal
activity provide an efficient way to ensure the quality of stored cereals, other
feed raw materials and compound feed (Celik et al., 2003). Organic acids
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(C1-C7) are widely distributed in nature as normal constituents of plants or
animal tissues. They are sometimes found as their sodium, potassium or
calcium salts or even as stronger double salts. Citric acid, fumaric acid,
propionic acid, lactic acid and formic acid are the commonly used acids in the
poultry diets.
2.6 PHYTASE AND CITRIC ACID SUPPLEMENTATION IN POULTRY DIET
2.6.1 Growth performance
Studies with chicks and turkeys have indicated a positive response in
growth performance from the addition of various organic acids to diets (Celik
et al., 2003; Owen et al., 2008). Gunes et al. (2001) and Adil et al. (2010) have
reported that the body weight gain was significantly improved by dietary
supplementation of organic acids when compared with the control group.
Yan et al. (2000) reported an increase in body weight at 21 day
in broilers with the addition of phytase. Many studies (Ahmad et al., 2000;
Pintar et al., 2004 and Bozkurt et al., 2006) have reported an increase in weight
gain with increasing concentration of dietary phytase in soybean meal based
diets. However, Pizzolante et al. (2002) have found no effect on weight gain of
broilers due to phytase addition. These differences among studies might have
resulted from the amount of available phosphorus used and amount of phytase
added in diets (Bingol et al., 2009).
Bingol et al. (2009) have observed that broilers fed negative control diet
had significantly lower feed efficiency compared with other treatment groups
that were supplemented with phytase. Bozkurt et al. (2006) noticed that feed
efficiency of broilers fed diet containing phytase were similar to those fed
control diet with adequate phosphate. Feed conversion ratio was found to be
better with phytase supplementation in broilers (Tejedor et al., 2001). Park et
al. (2009) and Sharafat et al. (2009) have reported better feed conversion ratio
when citric acid was added to the diet of layers. Omogbenigun et al. (2003)
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31
have noted a better feed conversion ratio in piglets when the diet was
supplemented with both phytase and organic acid.
The mortality rate observed during the study period was attributed to
phosphorus requirement. It was reported that not enough phosphorus was
available to the chicks (Sohail and Roland, 1999). Punna and Roland (1999)
have reported that phosphorus requirement of chicks varied with the age, size
and strain of birds. It was reported that phytase supplementation to moderate
and low nonphytate phosphorus level increased livability percentage
(Scheideler and Ferket, 2000).
The improvement in the performance of broilers fed with phytase
supplementation can be explained by the improved utilization of energy,
protein, amino acids, as well as macro and microminerals (Santos et al., 2008).
2.6.2 Mineral retention
Leeson and Summers (2001) stated that minerals are inorganic
materials occurring in nature in the form of salts or mixed with organic
compounds. The availability of minerals to animals and their metabolic
functions largely depend on the compound in which they are present.
Phosphorus, when combined with phytic acid is not available to monogastric
animals. Despite the adequacy of certain elements in the diet, deficiency
symptoms were observed at times.
Adding microbial phytase in combination with citric acid decreased the
phosphorus disappearance in the crop (a portion of the digestive system as
indicated in Figure 9) content compared to birds which were supplemented only
with phytase in laying hens (Ali et al., 2009). Viswanathan et al. (2007) have
also reported that 750 U of phytase plus 3% citric acid supplementation
improved the digestibility of phosphorus than control diet in pigs. Addition of
500 U microbial phytase/kg and 0.35% organic acid mixture composed mainly
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32
of citric acid improved phosphorus digestion and utilization, thereby leading to a
reduction in phosphorus excretion (Omogbenigun et al., 2003).
Viverous et al. (2002) had reported that compared to the normal
nonphytate phosphorus diet, the birds fed with low nonphytate phosphorus
diets without phytase had decreased calcium retentions at 3 (up to 30%) and 6
weeks of age (up to 25%). Phytase supplementation to the low nonphytate
phosphorus diets increased calcium retention at 3 weeks by 22% and 6 weeks
of age by 15%. Radcliffe et al. (1998) have reported that calcium digestibility
was improved by the addition of citric acid. Calcium retention was increased by
supplementation of both phytase and citric acid in broilers (Agustin et al.,
2003). The improvement in calcium availability has been expected because
phytase liberates calcium from the calcium-phytate complex and as the
availability of phosphorus increases, the availability of calcium also increases
(Ahmad et al., 2000).