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Sensors 2009, 9(9), 7038-7057; doi:10.3390/s90907038
Published: 4 September 2009
Abstract: In animal diets optimal amino acid quantities and balance among amino acids is of great nutritional importance. Essential amino acid deficiencies have negative impacts on animal physiology, most often expressed in sub-optimal body weight gains. Over supplementation of diets with amino acids is costly and can increase the nitrogen emissions from animals. Although in vivo animal assays for quantification of amino acid bioavailability are well established, Escherichia coli-based bioassays are viable potential alternatives in terms of accuracy, cost, and time input. E. coli inhabits the gastrointestinal tract and although more abundant in colon, a relatively high titer of E. coli can also be isolated from the small intestine, where primary absorption of amino acids and peptides occur. After feed proteins are digested, liberated amino acids and small peptides are assimilated by both the small intestine and E. coli. The similar pattern of uptake is a necessary prerequisite to establish E. coli cells as accurate amino acid biosensors. In fact, amino acid transporters in both intestinal and E. coli cells are stereospecific, delivering only the respective biological l-forms. The presence of free amino- and carboxyl groups is critical for amino acid and dipeptide transport in both biological subjects. Di-, tri- and tetrapeptides can enter enterocytes; likewise only di-, tri- and tetrapeptides support E. coli growth. These similarities in addition to the well known bacterial genetics make E. coli an optimal bioassay microorganism for the assessment of nutritionally available amino acids in feeds.
Biosensors make use of biological components to detect small amounts of chemicals or to characterize samples physiologically or chemically. The advantages of using these biologically based sensors lie in their specificity, sensitivity and portability. Also, unlike chemical or physical analyses, there is no need for large and expensive instrumentation. Biosensors can include enzymes or antibodies, but mainly microorganisms, especially bacteria, have been used. Bacteria have the capacity to grow rapidly in relatively inexpensive media.
The main application for microbial biosensors has been in the environmental area. Whole bacterial cells or sensor bacteria have been used by various research groups for analyzing different compounds, for example, inorganic mercury [1,2], naphthalene , and arsenite . Ivask et al.  reported on a sensor for organic mercury compounds that was constructed using Escherichia coli. Recently, the demand for quick and specific analytical tools for food and fermentation analysis has increased and is still expanding. Analyses have been developed for monitoring nutritional parameters, food additives, and food contaminants, among others. A common use for bacterial biosensors is for determination of sugars. Tkak et al.  used Gluconobacter oxydans as a biosensor for detecting total sugars in lignocellulose hydrolysates, and Rotariu et al.  used yeast cells for selective determination of sucrose. Escherichia coli has also been used as a sensor for sugars by Held et al. , who used it to detect both mono- and disaccharides. Likewise, a number of reports are available on microbial biosensors for specific amino acids such as tyrosine (Aeromonas phenologenes), tryptophan (Ps. fluorescens) and glutamic acid (B. subtilis) [9, 10]. In this review, the focus will be on the application of microbial biosensors for assessing amino acid bioavailability in animal feeds.
The concept of bioavailability is heavily relied on in animal nutrition to recognize the incomplete digestibility and utilization of proteins fed to animals . To compensate the incomplete digestibility of feed proteins and prevent nutritive deficiencies, diets are often supplemented with crystalline essential amino acids. However, if diets are not precisely formulated and amino acids are over-supplemented, excesses are not utilized for muscle development but released by excreta, thus becoming major substrates for ammonia production [9,10]. Ammonia is a colorless gas which is produced as a result of bacterial deamination or reduction of nitrogen substances in manure . An inventory of aerial pollutant emissions emanating from US poultry buildings estimated ammonia emissions to be 664,238 US tons/yr in 2002 . To decrease the level of ammonia emissions in poultry, the usage of diets with reduced and optimized nitrogen content has been recommended . Currently, protein level in feed diets is formulated based on the data for total amino acids. To assist the nutritionist in the preparation of efficient and low-price poultry diets and in the transition from total to bioavailable amino acids application, Applegate et al.  has suggested that information on both total and bioavailable values of essential amino acids be included on the labels of feed ingredients.
Although rapid and currently in use, chemical methods for the determination of amino acid levels in feed ingredients including high performance liquid chromatography (HPLC) and gas chromatography (GC) are not the most appropriate because they result in higher values than the amounts of amino acids utilized under physiological conditions . Currently, animal assays i.e. in vivo methods, are considered standard methods for the determination of bioavailable amino acids because obtained results represent the actual animal response to dietary treatments . These methods however, are very expensive, laborious, and time consuming . The development of alternative methods that are equally reliable but less complex and more rapid is desired. The purpose of this review is to describe and evaluate the theoretical basis of the possible use of Escherichia coli as a biosensor for determination of bioavailable amino acids in feed proteins. Major topics include discussion of E. coli as a natural inhabitant of the animal alimentary tract, comparison of amino acid/peptide assimilation by the small intestine and E. coli, and justification of the potential commercial applications for E. coli in the estimation of bioavailable amino acids in protein sources.
2. Microbial Biosensors for Amino Acid Quantification
As described by Shockman , microbial methods for quantification of biologically available amino acids are accurate, simple, specific and inexpensive. They involve different assay microorganisms (Table 1) and are based on their nutritive requirements for the respective amino acid. An additional requirement is the presence of either externally supplemented or internally expressed proteolytic activities of the assay microorganisms. Most microorganisms do not secrete extracellular proteolytic enzymes and, therefore, can be used for the assessment of only enzymatically pre-treated protein sources. Stott and Smith  and Bos et al.  used the protozoon Tetrahymena pyriformis in a protein quality evaluation of test materials mainly because of its proteolytic capabilities. It requires lysine to grow and therefore can be used for its quantification. However, a disadvantage of this microorganism is the relatively long incubation period (approximately four days). In addition, laborious and tedious cell count is the preferred method to measure the growth response to lysine. Other microorganisms such as Streptococcus faecalis, S. zymogenes, Leuconostoc mesenteroides, Pediococcus acidilactici, and Lactobacillus arabinosus have also been used in the determination of bioavailable amino acids (Table 1) [21–24]. Growth responses of these bacteria to the corresponding amino acids were measured by either optical density (OD) or titration of the produced lactic acid. The quantification of the latter was performed in the stationary phase of the microbial growth, taking approximately 72 h. Since other organic acids are also produced, the accuracy of the assay is influenced by whether total or lactic acid production is measured. In addition, lactic acid bacteria are characterized with relatively complex nutritive requirements which include vitamins, purine, and pyrimidine media supplementation to ensure optimal growth [18,25].
The most highly investigated microorganism for amino acid bioavailability quantification is Escherichia coli (Table 2). Although not naturally auxotrophic for amino acids like the lactic acid bacteria, E. coli has multiple advantages over other assay microorganisms . E. coli is characterized with the lowest doubling time among other bacteria . It is easy to grow and has simple media requirements. E. coli genetics is well established and can be easily manipulated to generate mutants with desired characteristics. Furthermore, E. coli is a part of the intestinal microflora of most animals and humans with presumably similar assimilation of amino acids and peptides which is a necessary prerequisite for the bacterium to serve as a biosensor microorganism for these compounds.
3. E. coli as a Gut Microorganism
The microflora of the gastrointestinal tract (GI) is diverse and complex. According to Moore and Holdeman , more than 400 bacterial species have been found in the colon. Gastrointestinal microflora play an important role in the determination of the total physical condition of animal species. The incredible variation in microbial population is determined by host physiology, environmental conditions, and microbial interactions. Mostly anaerobic but also aerobic as well as facultative anaerobic microorganisms have been isolated and characterized [29–31]. E. coli is a persistent inhabitant in the alimentary tract of both healthy and sick mammals [32,33] and can reach a level as high as 1010 bacterial cells per gram of fecal sample of an adult animal . As a facultative anaerobe it is capable of growing with minimal oxygen levels. This feature combined with its ability to survive over a relatively large range of pH makes it abundant even under conditions unfavorable for bacterial growth .
The overall population level of bacterial cells and in this particular case of those of E. coli along the GI tract is highly dependent on location. The human stomach is generally considered nearly sterile because of the low gastric pH . The small intestine is a transition zone between the stomach and the large intestine and contains a highly diverse and dense microbial population. The upper part of the small intestine is characterized by very low microbial counts with nearly complete absence of coliforms. In the distal ileum, gram negative bacteria outnumber gram positive and the coliform titer reaches 107 colony forming units (cfu)/mL. The reason E. coli does not inhabit the upper part of the small intestine may be due to an inability to adhere to the epithelium of the proximal tract and thus it is washed out at a rate that does not allow for persistent development in this zone . However, some pathogenic strains can adhere to the intestine because of their ability to produce lectins. For example, human enteropathogenic E. coli strains are found to bind to the human intestine. Puzstai et al.  observed adhesion of E. coli RDEC-1 to rabbit intestine.
The colonization of the intestine by E. coli strains producing K99 and F41 lectins is considered a major cause of neonatal diarrhea in calves . Interestingly, plant lectins found in diets, although not of bacterial origin, are also found to promote E. coli proliferation in the small intestine. According to Wilson et al. , coliform numbers increased from an initial count of approximately 103 cfu/g in small intestinal rat tissue to 1010 to 1011 within the first 24 to 48 hours of feeding a kidney bean diet. Although the upper part of the small intestine in healthy individuals is generally considered nearly free of coliforms, some studies from India  and South America  suggest the presence of enterobacteriaceae including E. coli and Klebsiella pneumonia in the upper intestines in healthy humans.
The large intestine is the part of the GI tract most heavily inhabited by microorganisms . While the abundance of E. coli in the colon is mainly associated with pathogenic consequences , this bacterium was found to be important in maintaining the diversity of indigenous microflora as well . By utilizing the oxygen diffused into the lumen, E. coli enables sensitive anaerobic bacteria to survive and participate in fermentative processes which are considered important for human health .
4. Protein Digestion in Animals. Small Intestine as the Primary Site for Amino Acid and Peptide Uptake
Proteins are major components of animals. The protein content of mature animals accounts for 15 to 18% of the body weight . The building blocks of proteins are amino acids that are either newly synthesized or derived from hydrolyzed food proteins. Protein digestion starts with the production of oligopeptides (containing more than three amino acids) in the animal stomach as a result of the direct exposure to pepsin which attacks peptide bonds involving aromatic amino acids. Oligopeptides are further hydrolyzed by pancreatic proteases along the digestive tract. Pancreatic proteases are divided into two major subgroups consisting of endopeptidases and exopeptidases. Endopeptidases including trypsin, chymotrypsin, and elastase are secreted into the duodenum as inactive precursors . After being transformed into active forms, they catalyze the disruption of endopeptide bonds thus releasing relatively large oligopeptides. External peptide bonds of polypeptides and proteins are digested by pancreatic exopeptidases. The complex hydrolysis action of pancreatic enzymes on feed proteins results in a mixture of free amino acids, di- and tripeptides and large peptides. The large peptides cannot be assimilated by the small intestine and must be further hydrolyzed by brush border-membrane peptidases . According to Johnson , luminal digestion of protein meal produces approximately 40% amino acids and 60% small peptides. The small intestine is the primary place where amino acids and small peptide absorption occurs although the absorptive capacity along the length of small intestine varies .
As an inhabitant of the small intestine without the capability to secrete extracellular proteases, E. coli is forced to assimilate the mixture of amino acids and peptides derived from the enzymatic degradation of food proteins [49,50]. This may lead to a competition between E. coli and the small intestine for protein digestive products as an eventual overgrowth of even non-pathogenic strains may slightly reduce the amount of nutrients available for the animal . Interestingly, although genetic and physiological differences between the prokaryotic E. coli and eukaryotic intestinal epithelial cells are considerable, the assimilation of the same compounds implies probable similarities in the mechanism of their absorption which is a must if E. coli is to be used as biosensor for bioavailable amino acid quantification [51,52].
5. Amino Acid and Peptide Transport in Small Intestine
Amino acids can enter the cells by simple diffusion, facilitated diffusion (Na+- independent), and active transport (Na+- dependent) [48,53]. The contribution of each transport system to the total amount of amino acids entering the cell is highly dependent on substrate concentration . The active transport is energetically expensive for cells. An amino acid is co-transported with a Na+ into the cell against the amino acid concentration gradient which requires additional energy input. It is provided by a membrane Na+ gradient which in turn is generated by a Na+/ K+-ATP dependent pump retaining low intracellular and high extracellular concentrations of Na+ . Because of the high energy expense, the active transportation of amino acids, in general, occurs at low extracellular concentrations. Stevens et al.  observed that phenylalanine enters the cells by active transport only at concentrations below 1 mmol/L. When leucine uptake was studied, it was reported that the combined active and facilitated diffusion contributed to leucine transport primarily at concentrations no higher than 5 mmol/L . For lysine and methionine, the active mechanism of transport occurred at an even lower concentration, namely 1.0 mmol/L . As the substrate concentration increases the contribution of facilitated transport and passive diffusion to the total amount amino acid uptake increases, implying simultaneous presence of several mechanisms for amino acid uptake. Most amino acids are transported by more than one transporter which provides not only high energy efficiency but also backup capacity for absorption in the case of mutational inactivation . Smith et al.  confirmed the presence of high-affinity and low-affinity carrier systems for serine, alanine, and methionine transport into rabbit ileal enterocytes. Bo-type Na+-dependent and Bo-type Na+-independent transporter systems for neutral amino acids have been characterized at the molecular level and reported to have a concentration-based mode of regulation [59–61].
The precise number of amino acid transport carriers is not known. Christensen  described 12 distinct amino acid transport systems. Stevens et al.  characterized and added three more intestinal amino acid carriers to the list. Although they differ in their location and kinetic characteristics, all of them have a common requirement for the possession of amino- (or imino-) and carboxyl groups by the substrate being transported . Based on this, Munck  concluded that intestinal carriers for amino acids can transport only amino acids.
Different transport systems exist for the import of small peptides. By studying intestinal amino acid and peptide transport in the rabbit ileum, Rubino et al.  established that free amino acids do not affect the transport of dipeptides and vice versa. Amino acid and peptide competition experiments have been used to confirm the existence of independent transport systems for amino acids and small peptides in intestines . The independent functions of amino acids and peptide carrier systems have been further demonstrated by studies performed with patients with deficiencies in amino acid metabolism such as Hartnup disease and cystinuria .
Since the Na+-dependent amino acid transport system was well understood, it was intuitively assumed that the same mechanism for peptide cell entry also occurred. However, by using brush-border membrane vesicles, Ganapathy et al.  demonstrated that peptide transport did not depend on Na+ gradient. Coupling of intracellular peptide concentration and H+ gradient was reported . Peptide transport in the small intestine driven by proton motive force was also confirmed by Miyamoto et al. . However, when dipeptide transport was studied in rabbit, rat, and human intestinal brush-border membrane vesicles (BBMV), Rejendran et al.  noted that generated proton motive force could not drive the accumulation of dipeptides against their concentration. Similar observations were reported by Wilson et al.  who studied tripeptide transport in human jejunal BBMV. In addition, the transport of glutathione in rabbit BBMV appeared to be energized by mono- and divalent (Ca2+) cations but not by H+ . Based on these conflicting data, Webb et al.  concluded that two classes of carrier-mediated peptide transporters exist: one that is energized by proton motive force, and another that is energized by cations other than H+ and Na+.
Regardless of the mechanisms for the entry of peptides into the cells however, only di- and tri-peptides can be transported by carriers . One of the methods most widely used to determine the maximal number of amino acid residues for peptide absorption was based on peptide disappearance from the gut lumen in the presence of specific inhibitors of brush border peptide hydrolases . Using such a method, Adibi  concluded that only di- and tri-peptides are actively transported by carriers in the small intestine with very low probability for tetrapeptides to actively cross the cell membrane. Instead, they are hydrolyzed to free amino acids and smaller peptides by brush border peptidases .
Except for the number of amino acid residues in peptides, the presence of amino and carboxyl terminal groups appeared to be critical for peptide uptake. Addison et al.  observed that the blocking of N-terminal group by acetylation or methylation or the C-terminal group by esterification highly decreased the peptide affinity for transporters. Cyclization of dipeptides was a different approach to evaluate the importance of terminal amino- and carboxyl groups . Subsequent experiments demonstrated that cyclic dipeptides failed to compete with the corresponding linear dipeptides as evidenced by their substrate affinity constants.
Stereospecificity of dipeptide transporters has also been studied as an important characteristic. Asatoor et al.  observed that the absorption rate of l-Ala-l-Phe and l-Leu-l-Leu is much greater than those of their respective d-d isomers. A thorough investigation on the stereospecifity of kidney oligopeptide/H+ symporter was performed by Daniel et al. . The research group established 60-fold reduction in the transporter affinity when l-Ala in Ala-Gly dipeptide was substituted by its d-isomer. The replacement of –COOH terminal residue with its d-isomer led to even greater reduction in the affinity. The substitution of both l-amino acids with their d-forms completely abolished the uptake of the dipeptide. Although they observed less reduction in the substrate affinity of lipophilic peptides with d-amino acid substitutes, the overall conclusion was that the peptide stereospecifity was an important determinant of transporter affinity. Since the biologically active form of amino acids is the l-form and only l-amino acids are utilized for the synthesis of new proteins, these observations were not surprising .
6. Comparative Characteristics of Amino Acid and Peptide Transport in E. coli
The overall comparison of amino acid and peptide transport in E. coli and animal small intestine is outlined in Table 3. E. coli can synthesize all of the amino acids from inorganic compounds and glucose but it is also capable of transporting intact amino acids into the cell from the extracellular environment. For E. coli, the amino acids can serve as a sole carbon or nitrogen source. However, the catabolism of amino acids is energetically expensive and in a natural environment such as the small intestine, where other carbon sources are also available, the uptake of amino acids is designed to replenish the intracellular pool of amino acids necessary for the biosynthesis of proteins, nitrogen transfer, or osmotic protection [50,80,81].
As in the small intestinal epithelial cells, there are three ways for amino acids to enter the bacterial cells: passive diffusion, facilitated diffusion and active transport . Passive diffusion and facilitated diffusion do not require additional energy input as they occur at relatively high concentrations of substrates. However, active transporters are activated at low concentrations of substrates with a Michaelis-Menten (Km) constant varying in the range of 1 to 10 μM . Some high affinity transporters such as for l-glutamine and l-proline were reported to have even lower Km, namely 0.1 and 0.7 μM respectively .
Just as with intestinal transporters, microbial active uptake systems require energy input since substrates are transported against their concentration gradient. Common energy sources for the active transport in bacterial cells are H+- and Na+ -membrane concentration gradients, and ATP hydrolysis. While in the small intestine active transport of amino acids is dependent mostly on the Na+-membrane gradient , in E. coli, all three energy sources can be used depending on transporters and amino acid (s) being transported. The specific tyrosine and leucine transporters are energized by H+-membrane gradients , while the ABC transporters for aromatic amino acids and hystidine are energized by ATP hydrolysis . Although the Na+-membrane gradient is not considered typical for prokaryotes, the transport of L-serine and L-threonine  as well as those of proline  is considered Na+-dependent.
Based on kinetic analysis, several distinct transport systems for amino acids with very little overlap have been described in E. coli . Distinct transport systems exist for branched amino acids (isoleucine, leucine and valine) and aromatic amino acids (tyrosine, phenylalanine and tryptophan). Distinguishable transport systems for hystidine and proline have also been described. In addition, multiple transporters may exist for the amino acids belonging to one group [85, 88]. They differ mainly in their affinity to the substrates and are regulated by the intracellular level of the respective compound. For example, the low affinity transport system (LIV-II) for the branched amino acids usually operates under optimal concentrations of the respective substrates, while the high affinity carrier is activated by leucine starvation. A third system, specific only for the transport of leucine, also exists and is considered a component of the branched chain amino acid family transport system . There are two systems for lysine, ornithine, and arginine  as well as for aspartate and glutamine . Five transporters for the intracellular accumulation of aromatic amino acids have been identified and studied . In short, the diversity in the transport systems for amino acids in E. coli is much higher than the uptake systems in the small intestine of the host. The reason for this may relate to the requirements for bacterial populations to meet their physiological needs under different environmental conditions that are unfavorable for their growth. Regardless of these differences, a common feature of amino acid transport in both small intestine and E. coli is the transport of amino acids by active mechanisms at low substrate concentrations and the stereospecifity of transporters. As Piperno and Oxender  stated, all amino acid transporters except for those of alanine, glycine and serine, are highly stereospecific, being able to transport only l-amino acids.
E. coli absorb not only free amino acids but also small peptides. As in the small intestine, there are distinct transport systems for the import of amino acids and peptides [82,91]. The isolation of mutants deficient in transport system in either of them as well as the experiments involving competitive inhibition between amino acids and dipeptides unambiguously proved the independent existence of amino acid and dipeptide transport . E. coli dipeptide transport resembles that of the small intestine in its specific requirement for N- and C-terminal groups and the blockage of these functional groups prevents dipeptide uptake . Like intestinal transporters, E. coli dipeptide transport systems are also highly stereospecific, the reason potentially being the inability of E. coli to convert d-stereoisomers into utilizable l-forms .
The difference in the peptide utilization by small intestine and E. coli cells is the existence of a distinct oligopeptide system. The oppABCDF system is located at 27 min of the E. coli genome and is able to transport peptides containing from two to five amino acid residues [93,94]. However, it appeared that the Opp was specifically capable of transporting and recycling exclusively cell wall peptides which may explain the existence of this transporter in E. coli but not in intestinal cells . These findings agreed with previous observations that some oligopeptides, although satisfying the structural requirements for oligopeptide transport, were unable to enter E. coli cells . While tetrapeptides of lysine and arginine poorly supported E. coli growth, pentapeptides and higher homologues completely abolished the bacterial propagation .
Consistent with other active transports, peptide transport in E. coli requires energy. While in the small intestine proton motive force is considered a primary energy source, in E. coli cells this role is assigned to ATP hydrolysis [97–99]. ATP hydrolysis occurs concomitantly with the function of periplasmic binding protein-dependent transport systems including Opp which are considered to play a major role in peptide transport in E. coli [100–102]. By studying the transport of Opp-specific substrate l-prolylglycylglycine, Mimmack et al.  recorded ATP consumption in the wild type strain but not in the opp− mutant. In addition, proton motive force (pmf) was discovered to take part in peptide transport as well . It seems however, that pmf-dependent systems were specific only for the transport of di- and tripeptides .
Although E. coli and intestinal cells are structurally very different, it appears that substantial similarities in amino acid and peptide uptake between both biological subjects exist. In fact, amino acid transporters in both intestinal and E. coli cells are stereospecific, delivering only the respective biological l-forms. The presence of free amino- and carboxyl groups is critical for amino acid and dipeptide transport. Di-, tri- and tetrapeptides can enter enterocytes; only di-, tri- and tetrapeptides support E. coli growth. These similarities along with other specific characteristics are very important prerequisites for a test microorganism to achieve an optimal correlation between potential microbiological assays and the corresponding animal assays currently in use for amino acid bioavailability quantification.
7. E. coli in Use as a Biosensor to Assess Amino Acid Bioavailability in Feed Proteins
Animal assays, i.e. in vivo methods, are considered standard methods for the determination of bioavailable amino acids because the results obtained represent the actual animal response to dietary treatments . Although accurate and reliable, they are laborious, time consuming, and expensive to be used on a daily basis. In contrast, microbiological assays do not require elaborate instrumentation. They are simple, specific and inexpensive. To be used as a test microorganism, a bacterium should be an auxotroph i.e. it should be deficient for the amino acid of interest. The cell growth of such an auxotroph is a direct function of the concentration of the compound being assayed . Therefore, the amount of the amino acid in the medium can be determined by measuring bacterial cell growth. Wild type E. coli can synthesize all 20 amino acids growing in medium containing only a carbon source and inorganic salts. Consequently, the wild type E. coli cannot be used directly for amino acid quantification. Although not a natural auxotroph for amino acids, E. coli has multiple advantages over other assay microorganisms. It is easy to grow and it does not require elaborate equipment and expensive nutritive ingredients. In addition, E. coli is characterized with the lowest doubling time among other bacteria which determines the relatively short time (7 to 8 h) required to reach stationary phase . E. coli genetics is well established and can be easily manipulated. Multiple mutants have been created and studied for the purpose of bioavailable amino acid quantification (Table 2).
The extensive research towards the development of a stable lysine auxotroph strain is determined by the limiting amount of this amino acid in feed ingredients and the high variability of its bioavailability . The accurate measurement of bioavailable lysine in feed ingredients would prevent the addition of lysine in excess as a “safety factor” used in the animal practice to compensate the uncertainty about lysine bioavailability and the animal requirement for this nutrient . The diversity of the detection modes used in these types of assays is also presented in Table 2. With the discovery and the application of green fluorescent protein (GFP) as a reporter [108,109], the potential of E. coli assays for rapid and accurate estimation of bioavailable lysine even under non-sterile conditions increased . Finally, as a gastrointestinal microorganism competing with intestinal cells for some dietary derived amino acids and peptides available in the animal gut, E. coli appear to be a promising alternative to test animals used in the quantification of bioavailable amino acids.
The idea of using E. coli to assay accurately bioavailable amino acids in proteins was suggested by Gilvarg and Katchalski  and later by Payne , who showed that there were no differences in E. coli lysine auxotroph growth responses to either free lysine or lysine in peptide linkage of di- and tripeptides. This observation enabled bioavailable lysine (free lysine, di- and tri- lysine containing peptides) to be evaluated simply by the construction of a crystalline lysine standard curve. Since E. coli does not naturally excrete extracellular proteases and peptidases, an enzymatic pre-digestion of a protein is required for an in vitro analysis. Therefore, the successful use of E. coli to assay bioavailable amino acids in feed proteins was dependent on the development of a pre-digestion procedure that closely simulated the in vivo protein digestion occurring in the gastrointestinal tract. A variety of single enzymes and enzyme combinations have been explored to degrade feed proteins to an amino acid/peptide mixture that mimics the in vivo digestive protein product. Payne et al.  reported that among pepsin, trypsin, chymotrypsin, pronase and peptidase, the combination of pronase and peptidase was the best for the estimation of bioavailable lysine in proteins when using an E. coli lysine auxotroph. By exploring the digestive profiles of the studied protein sources, they established that the combination of pronase and peptidase released only negligible amounts of oligopeptides larger than pentalysine which was an important prerequisite due to the size requirements for the digestive products. Protein cleavage products should be small enough to pass the bacterial cell wall and reach their cytoplasmic carriers if E. coli is to be used as a test microorganism [49,111]. When Erickson et al.  used both pronase and peptidase to pre-digest animal protein feeds, they obtained a correlation of 0.94 between lysine bioavailability determined by using E. coli lysine auxotrophs and previously published chick bioassay data. Following the same procedure but measuring the fluorescence emission of an E. coli lysine auxotroph transformed with a gfpmut3, Chalova et al. [113,114] were able to determine bioavailable lysine in feed proteins including sorghum, soybean meal, cotton seed meal, meat and bone meal, chick starter and finisher, and swine starter in a 6-hour period. No significant differences in estimated bioavailable lysine were observed when data were compared to the data for bioavailable lysine generated by chick bioassay on the same feed samples except for sorghum.
An E. coli methionine auxotroph was used to quantify bioavailable methionine in protein sources . The strain was transformed with a plasmid carrying a gene for a green fluorescent protein. Bacterial growth response to the protein derived methionine was measured either turbidimetrically or by fluorescence. The method was also adapted for application using microtiter plates which not only decreased the time required for an assay completion if compared to tube-based assays but also diminished material and equipment expenses . Microbial E. coli based assays for determination of bioavailable amino acids in protein sources performed in microtiter plates highly reduced the volume of media and incubation space required and enabled simultaneous quantification of a large number of samples.
Methionine and lysine bioavailability in foods were also quantified by Hitchins et al. . Their method was based on the study of Tuffnell et al.  who observed that the extent of the synthesis of β-galactosidase strictly depends on the externally supplemented lysine. Following the same procedure, Hitchins et al.  determined the bioavailability of cysteine, threonine and tryptophan by measuring the activity of β-galactosidase in 17 pronase digested foods. They concluded that the method was reliable and accurate enough to predict the first and second limiting amino acid.
In conclusion, E. coli can be considered a promising test microorganism for the evaluation of bioavailable amino acids in protein sources. The intrinsic properties of these bacteria as well as the numerous similarities between protein digestion product assimilation by E. coli and the small intestine make the development of accurate and reliable microbial methods for bioavailable amino acid quantification possible. The time required for the completion of the microbial assay (6–8 hours) [110,119] is much less than the time required for the chick bioassay (two to three weeks) [17,113,120]. Based on the current results published in literature, the microbial assay appears to have other advantages as well. Factors such as low metabolizable energy and low amino acid content of feed samples do not affect E. coli assays while they are of serious consideration if an animal assay is to be used for those sample analyses . Environmental temperature, sex, age and species highly influence the animal response to the amino acids as well . In addition, animal methods are not suitable for the generation of high through-put volumes of data because only one amino acid can be measured at a time. However, E. coli auxotrophs for different amino acids could be generated and corresponding biosensors developed for the estimation of a large set of nutritionally important amino acids. The different strains could be applied simultaneously using microtiter plates and the bioavailability of all essential amino acids in protein sample(s) determined.
This review was supported by Hatch grant H8311 administered by the Texas Agricultural Experiment Station and Texas Advanced Technology Program, grant #: 000517-0220-2001 (Texas Higher Education Board, Austin, TX, USA).
- Seliffonova, O.; Burlage, R.; Barkay, T. Bioluminescent sensors for detection of bioavailable Hg (II) in the environment. Appl Environ. Microbiol 1993, 59, 3083–3090.
- Virta, M.; Lampinen, J.; Karp, M. A luminescence-based mercury biosensor. Anal. Chem 1995, 67, 667–669.
- King, J.M.H.; DiGrazia, P.M.; Applegate, B.; Burlage, R.; Sanseverino, J.; Dunbar, P.; Larimer, F.; Sayler, G.S. Rapid, sensitive bioluminescent reporter technology for naphthalene exposure and biodegradation. Science 1990, 249, 778–781.
- Ramanathan, S.; Shi, W.; Rosen, E.P.; Daunert, S. Sensing antimonite and arsenite at the subattomole level with genetically engineered bioluminescent bacteria. Anal. Chem 1997, 69, 3380–3384.
- Ivask, A.; Hakkila, K.; Virta, M. Detection of organomercurials with sensor bacteria. Anal. Chem 2001, 73, 5168–5171.
- Tkac, J.; Gemeiner, P.; Svitel, J.; Benikovsky, T.; Sturdik, E.; Vala, V.; Petrus, L.; Hrabarova, E. Determination of total sugars in lignocellulose hydrolysate by a mediated Gluconobacter oxydans biosensor. Anal. Chim. Acta 2000, 420, 1–7.
- Rotariu, L.; Bala, C.; Magearu, V. Use of yeast cells for selective determination of sucrose. Rev. Roum. Chim 2000, 45, 21–26.
- Johnson, R.J. Principles, problems and application of amino acid digestibility in poultry. World’s Poult. Sci. J 1992, 48, 232–246.
- Verstegen, M.W.A.; Jongbloed, A.W. Crystalline amino acids and nitrogen emission. In Amino Acids in Animal Nutrition; D’Mello, J.P.F., Ed.; CABI Publishing: Wallingford, UK, 2003; p. 449.
- Kim, W.K.; Froelich, C.A., Jr.; Patterson, P.H.; Ricke, S.C. The potential to reduce poultry nitrogen emissions with dietary methionine or methionine analogues supplementation. World’s Poult. Sci. J 2006, 62, 338–353.
- Ritz, C.W.; Fairchild, B.D.; Lacy, M.P. Implications of ammonia production and emissions from commercial poultry facilities: A review. J. Appl. Poult. Res 2004, 13, 684–692.
- EPA. National emission inventory—Ammonia emissions from animal husbandry operations. http://www.epa.gov/ttnchie1/ap42/ch09/related/nh3inventorydraft_jan2004.pdf (accessed on August 14, 2009).
- Chambers, B.J.; Smith, K. Nitrogen: some practical solutions for the poultry industry. World’s Poult. Sci. J 1998, 54, 353–357.
- Applegate, T.; Thompson, K.; Dudley-Cash, W.A. Amino acid digestibilities needed for poultry rations. Feedstuffs 2004, 76, 15–17.
- Kivi, J.T. Amino acids. In Food analysis by HPLC; Marcel Dekker Inc: New York, NY, USA, 2000; p. 55.
- France, J.; Theodorou, M.K.; Lowman, R.S.; Beever, D.E. Feed evaluation for animal production. In Feeding Systems and Feed Evaluation Models; Theodorou, M.K., France, J., Eds.; CABI Publishing: Wallingford, UK, 2000; p. 1.
- Nordheim, J.P.; Coon, C.N. A comparison of four methods for determining available lysine in animal protein meals. Poult. Sci 1984, 63, 1040–1051.
- Shockman, D. Amino acids. In Analytical microbiology; Kavanagh, F., Ed.; Academic Press: New York, NY, USA, 1963; p. 567.
- Stott, J.A.; Smith, H. Microbiological assay of protein quality with Tetrahymena pyriformis W .4. Measurement of available lysine, methionine, arginine and histidin. Br. J. Nutr 1966, 20, 663–673.
- Bos, C.; Gaudichon, C.; Tome, D. Nutritional and physiological criteria in the assessment of milk protein quality for humans. J. Am. Coll. Nutr 2000, 19, S191–S205.
- Cardinal, E.V.; Hedrick, L.R. Microbiological assay of corn steep liquor for amino acid content. J. Biol. Chem 1948, 172, 609–612.
- Blackmore, J.A.; Parry, T.E. Microbiological assay of amino acids in serum: valine, leucine, and methionine. J. Clin. Path 1972, 25, 171–175.
- Wells, P.; McDonough, F.; Bodwell, C.E.; Hitchens, A. The use of Streptococcus zymogenes for estimating tryptophan and methionine bioavailability in 17 foods. Plant Foods Hum. Nutr 1989, 39, 121–127.
- Odunfa, S.A.; Adeniran, S.A.; Teniola, O.D.; Nordstrom, J. Evaluation of lysine and methionine production in some lactobacilli and yeasts from Ogi. Int. J. Food Microbiol 2001, 63, 159–163.
- Barton-Wright, E.C. The microbiological assay of the “essential” amino-acids in compound feedingstuffs. Analyst 1972, 97, 138–141.
- Payne, J.W.; Tuffnell, J.M. Assays for amino acids, peptides and proteins. In Microorganisms and nitrogen sources; Payne, J.W., Ed.; John Wiley & Sons: New York, NY, USA, 1980; p. 727.
- Ingraham, J.L.; Maaløe, O.; Neidhardt, F.C. Growth of the Bacterial Cell; Sinauer Associates, Inc: Sunderland, MA, USA, 1983.
- Moore, W.E.C.; Holdeman, L.V. Discussion of current bacteriologic investigations of the relationships between intestinal flora, diet and colon cancer. Cancer Res 1975, 35, 3418–3420.
- Simon, L.G.; Gorbach, L.S. Intestinal flora in health and disease. In Physiology of the Gastrointestinal Tract; Johnson, L., Ed.; Raven Press: New York, NY, USA, 1981; Volume 2, p. 1361.
- Gibson, G.R. Dietary modulation of the human gut microflora using the prebiotics oligofructose and inulin. J. Nutr 1999, 129, S1438–S1441.
- Vernazza, C.L.; Gibson, G.R.; Rastall, R.A. Carbohydrate preference, acid tolerance and bile tolerance in five strains of Bifidobacterium. J. Appl. Microbiol 2006, 100, 846–853.
- Mansfield, K.G.; Lin, K.; Newman, J.; Schauer, D.; MacKey, J.; Lackner, A.A.; Carville, A. Identification of enteropathogenic Escherichia coli in simian immunodeficiency virus-infected infant and adult rhesus macaques. J. Clin. Microbiol 2001, 39, 971–976.
- Irlbeck, N.A. How to feed the rabbit (Oryctolagus cuniculus) gastrointestinal tract. J. Anim. Sci 2001, 79, E343–346.
- Tannock, W.G. The acquisition of the normal microflora of the gastrointestinal tract. In Human health: the contribution of microorganisms; Gibson, S., Ed.; Springer-Verlag: London, UK, 1994; p. 1.
- Ingraham, J.L.; Marr, A.G. Effect of temperature, pressure, pH, and osmotic stress on growth. In Escherichia coli and Salmonella. Cellular and molecular biology; Neidhardt, F.C., Curtiss, R., III, Ingraham, J.L., Lin, E.C.C., Low, K.B., Magasanik, B., Reznikoff, W.S., Riley, M., Schaechter, M., Umbarger, H. E., Eds.; ASM Press: Washington, DC, USA, 1996; Volume 2, p. 1570.
- Finegold, M.S.; Sutter, L.V.; Mathisen, E.G. Normal indigenous intestinal flora. In Human intestinal microflora in health and disease; Hentges, D., Ed.; Academic Press: New York, NY, USA, 1983; p. 3.
- Puzstai, A.; Grant, G.; King, P.T.; Clarke, W.M.E. Chemical probiosis. In Recent advances in animal nutrition; Haresign, W., Cole, D.J.A., Eds.; Butterworths: London, UK, 1990; p. 47.
- Gaastra, W.; de Graaf, F.K. Host-specific fimbrial adhesins of noninvasive enterotoxigenic Escherichia coli strains. Microbiol. Mol. Biol. Rev 1982, 46, 129–161.
- Wilson, A.B.; King, T.P.; Clarke, E.M.; Pusztai, A. Kidney bean (Phaseolus vulgaris) lectin-induced lesions in rat small intestine: 2. Microbiological studies. J. Comp. Pathol 1980, 90, 597–602.
- Bhat, P.; Shantakumari, S.; Rajan, D.; Mathan, V.L.; Kapadia, C.R.; Swarnabai, C.; Baker, S.J. Bacterial flora of the gastrointestinal tract in Southern Indian control subjects and patients with tropical sprue. Gastroenterology 1972, 62, 11–21.
- Cain, J.R.; Mayoral, L.G.; Lotero, H.; Bolanos, O.; Duque, E. Enterobacteriaceae in the jejunal microflora prevalence and relationship to biochemical and histological evaluations in healthy Colombian men. Am. J. Clin. Nutr 1976, 29, 1397–1403.
- Macfarlane, S.; Dillon, J.F. Microbial biofilms in the human gastrointestinal tract. J. Appl. Microbiol 2007, 102, 1187–1196.
- Bronowski, C.; Smith, S.L.; Yokota, K.; Corkill, J.E.; Martin, H.M.; Campbell, B.J.; Rhodes, J.M.; Hart, C.A.; Winstanley, C. A subset of mucosa-associated Escherichia coli isolates from patients with colon cancer, but not Crohn's disease, share pathogenicity islands with urinary pathogenic E. coli. Microbiology 2008, 154, 571–583.
- Savage, D.C. Microbial ecology of the gastrointestinal tract. Annu. Rev. Microbiol 1977, 31, 107–133.
- Riis, P.M. The role of tissue constituents and products: proteins. In World animal science. A3. Dynamic biochemistry of animal production; Riis, P.M., Ed.; Elsevier: Amsterdam, The Netherlands, 1983; p. 75.
- Pizauro, J.M., Jr.; Ferro, J.A.; de Lima, A.C.F.; Routman, K.S.; Portella, M.C. The zymogen-enteropeptidase system: A practical approach to study the regulation of enzyme activity by proteolytic cleavage. Biochem. Mol. Biol. Edu 2004, 32, 45–48.
- Johnson, L.R. Digestion and absorption. In Gastrointestinal physiology; Johnson, L., Ed.; Mosby: St. Louis, MO, USA, 2001; p. 119.
- Webb, K.E., Jr. Intestinal absorption of protein hydrolysis products: a review. J. Anim. Sci 1990, 68, 3011–3022.
- Payne, J.W.; Bell, G.; Higgins, F. The use of Escherichia coli Lys− auxotroph to assay nutritionally available lysine in biological materials. J. Appl. Bacteriol 1977, 42, 165–177.
- McFall, E.B.; Newman, B.E. Amino acids as carbon sources. In Escherichia coli and Salmonella: Cellular and molecular biology; Neidhardt, F.C., Curtiss, R., III, Ingraham, J.L., Lin, E.C.C., Low, K.B., Magasanik, B., Reznikoff, W.S., Riley, M., Schaechter, M., Umbarger, H.E., Eds.; ASM Press: Washington, DC, USA, 1996; Volume 1, p. 358.
- Matthews, D.M. Introduction. In Peptide transport and hydrolysis, CIBA Foundation Symposiu. No. 50,; Elsevier: Amsterdam, The Netherlands, 1977; p. 5.
- Matthews, D.M.; Payne, J.W. Peptides in the nutrition of microorganisms and peptides in relation to animal nutrition. In Peptide transport in protein nutrition; Matthews, M.D., Payne, W.J., Eds.; North-Holland Publishing Co: Amsterdam, The Netherlands, 1975; p. 1.
- Krehbiel, C.R.; Matthews, J.C. Absorption of amino acids and peptides. In Amino acids in animal nutrition; D’Mello, J.P.F., Ed.; CABI Publishing: Wallingford, UK, 2003; p. 41.
- Stevens, B.R.; Kaunitz, J.D.; Wright, E.M. Intestinal transport of amino acids and sugars: advances using membrane vesicles. Annu. Rev. Physiol 1984, 46, 417–433.
- Wolffram, S.; Eggenverger, E.; Scharrer, E. Kinetics of D-glucose and L-leucine transport into sheep and pig intestinal brush-border membrane vesicles. Comp. Biochem. Physiol 1986, 84A, 589–593.
- Wilson, J.W.; Webb, K.E., Jr. Lysine and methionine transport by bovine jejunal and ileal brush border membrane vesicles. J. Anim. Sci 1990, 68, 504–514.
- Bröer, S. Amino acid transport across mammalian intestinal and renal epithelia. Physiol. Rev 2008, 88, 249–286.
- Smith, W.M.; Sepúlveda, V.F.; Paterson, F.Y.J. Cellular aspects of amino acid transport. In Intestinal transport: fundamental and comparative aspects; Gilles-Baillien, M., Gilles, R., Eds.; Springer: Berlin, Germany, 1983; p. 46.
- Lee, W.; Hawkins, R.; Peterson, D.; Vina, J. Role of oxoproline in the regulation of neutral amino acid transport across the blood-brain barrier. J. Biol. Chem 1996, 271, 19129–19133.
- Bröer, S.; Cavanaugh, J.A.; Rasko, J.E.J. Neutral amino acid transport in epithelial cells and its malfunction in Hartnup disorder. Biochem. Soc. Trans 2005, 33, 233–236.
- Ristic, Z.; Camargo, S.M.R.; Romeo, E.; Bodoy, S.; Bertran, J.; Palacin, M.; Makrides, V.; Furrer, E.M.; Verrey, F. Neutral amino acid transport mediated by ortholog of imino acid transporter SIT1/SLC6A20 in opossum kidney cells. Am. J. Physiol. Renal Physiol 2006, 290, F880–F887.
- Christensen, H.N. Organic ion transport during seven decades the amino acids. Bioch. Biophys. Acta 1984, 779, 255–269.
- Schultz, G.S.; Yu-Tu, L.; Strecker, C.K. Influx of neutral amino acids across the brush border of rabbit ileum. Stereospecifity and the roles of the α-amino and α-carboxylate groups. Biochim. Biophys. Acta 1972, 288, 367–379.
- Munck, G.B. Intestinal absorption of amino acids. In Physiology of the gastrointestinal tract; Johnson, L., Ed.; Raven Press: New York, NY, USA, 1981; Volume 2, p. 1097.
- Rubino, A.; Field, M.; Shwachman, H. Intestinal transport of amino acid residues of dipeptides. 1. Influx of the glycine residue of glycyl-l-proline across mucosal border. J. Biol. Chem 1971, 246, 3542–3548.
- Silk, D.B.A.; Grimble, G.K.; Rees, R.G. Protein digestion and amino acid and peptide absorption. Proc. Nutr. Soc 1985, 44, 63–72.
- Ganapathy, V.; Mendicino, J.; Leibach, F. Transport of glycyl-L-proline into intestinal and renal brush border vesicles from rabbit. J. Biol. Chem 1981, 256, 118–124.
- Takuwa, N.; Shimada, T.; Matsumoto, H.; Hoshi, T. Proton-coupled transport of glycylglycine in rabbit renal brush-border membrane vesicles. Bioch. Biophys. Acta 1985, 814, 186–190.
- Miyamoto, Y.; Ganapathy, V.; Leibach, F.H. Proton gradient-coupled uphill transport of glycylsarcosine in rabbit renal brush-border membrane vesicles. Biochem. Biophys. Res. Commun 1985, 132, 946–953.
- Rajendran, V.M.; Harig, J.M.; Ramaswamy, K. Characteristics of glycyl-L-proline transport in intestinal brush-border membrane vesicles. Am. J. Physiol. Gastrointest. Liver Physiol 1987, 252, G281–G286.
- Wilson, D.; Barry, J.A.; Ramaswamy, K. Characteristics of tripeptide transport in human jejunal brush-border membrane vesicles. Bioch. Biophys. Acta - Biomembranes 1989, 986, 123–129.
- Vincenzini, M.T.; Iantomasi, T.; Favilli, F. Glutathione transport across intestinal brush-border membranes: effects of ions, pH, Δψ, and inhibitors. Bioch. Biophys. Acta 1989, 987, 29–37.
- Webb, K.E., Jr.; Matthews, J.C.; DiRienzo, D.B. Peptide absorption: a review of current concepts and future perspectives. J. Anim. Sci 1992, 70, 3248–3257.
- Adibi, S.; Kim, Y. Peptide absorption and hydrolysis. In Physiology of gastrointestinal tract; Johnson, L., Ed.; Raven Press: New York, NY, USA, 1981; Volume 2, p. 1073.
- Adibi, S.A.; Morse, E.L.; Masilamani, S.S.; Amin, P.M. Evidence for two different modes of tripeptide disappearance in human intestine. Uptake by peptide carrier systems and hydrolysis by peptide hydrolases. J. Clin. Invest 1975, 56, 1355–1363.
- Addison, M.; Burston, D.; Payne, J.; Wilkinson, S.; Matthews, M. Evidence for active transport of tripeptides by hamster jejunum in vitro. Clin. Sci. Mol. Med 1975, 46, 707–714.
- Daniel, H.; Morse, E.; Adibi, S. Determinants of substrate affinity for the oligopeptide/H+ symporter in the renal brush border membrane. J. Biol. Chem 1992, 267, 9565–9573.
- Asatoor, A.M.; Chadha, A.; Milne, M.D.; Prosser, D.I. Intestinal absorption of stereoisomers of dipeptides in the rat. Clin. Sci. Mol. Med 1973, 42, S199–S212.
- Eastwood, M. Basic nutrients. In Principles of human nutrition; Eastwood, M., Ed.; Chapman & Hall: London, UK, 1997; p. 105.
- Reitzer, L. Ammonia assimilation and the biosynthesis of glutamine, glutamate, aspartate, asparagines, L-alanine and D-alanine. In Escherichia coli and Salmonella: Celular and molecular biology; Neidhardt, F.C., Ed.; ASM Press: Washington, DC, USA, 1996; p. 391.
- Trinidad, T.P.; Wolever, T.M.S.; Thompson, L.U. Availability of calcium for absorption in the small intestine and colon from diets containing available and unavailable carbohydrates: an in vitro assessment. Int. J. Food Sci. Nutr 1996, 47, 83–88.
- Sussman, A.J.; Gilvarg, C. Peptide transport and metabolism in bacteria. Annu. Rev. Biochem 1971, 40, 397–408.
- Piperno, J.R.; Oxender, D.L. Amino acid transport systems in Escherichia coli K12. J. Biol. Chem 1968, 243, 5914–5920.
- Eze, M.O.; McElhaney, R.N. Effects of temperature on active amino acid transport in Escherichia coli strain 7. Microbios 1989, 58, 173–182.
- Antonucci, T.K.; Oxender, D.L. The molecular biology of amino-acid transport in bacteria. Adv. Microb. Physiol 1986, 28, 145–180.
- Hosie, A.H.F.; Poole, P.S. Bacterial ABC transporters of amino acids. Res. Microbiol 2001, 152, 259–270.
- Hama, H.; Shimamoto, T.; Tsuda, M.; Tsuchiya, T. Properties of a Na+-coupled serine-threonine transport system in Escherichia coli. Biochim. Biophys. Acta 1987, 905, 231–239.
- Haney, S.; Oxender, D. Amino acid transport in bacteria. Intern. Rev. Cytol 1992, 137A, 37–95.
- Steffes, C.; Ellis, J.; Wu, J.; Rosen, B.P. The lysP gene encodes the lysine-specific permease. J. Bacteriol 1992, 174, 3242–3249.
- Koyanagi, T.; Katayama, T.; Suzuki, H.; Kumagai, H. Identification of the LIV-I/LS system as the third phenylalanine transporter in Escherichia coli K-12. J. Bacteriol 2004, 186, 343–350.
- Payne, J.W. Transport of peptides in bacteria. In Bacterial transport; Rosen, B., Ed.; Marcel Dekker, Inc: New York, NY, USA, 1978; Volume 4, p. 325.
- Payne, J.W. Transport of peptides in microorganisms. In Peptide transport in protein nutrition; Matthews, M.D., Payne, J.W., Eds.; Elsevier: Amsterdam, The Netherlands, 1975; p. 283.
- Payne, J.W. Peptide transport in bacteria: methods, mutants and energy coupling. Bioch. Soc. Trans 1983, 11, 794–798.
- Andrews, J.C.; Short, S.A. opp-lac operon fusions and transcriptional regulation of the Escherichia coli trp-linked oligopeptide permease. J. Bacteriol 1986, 165, 434–442.
- Higgins, C.F. Peptide transport systems of Salmonella Typhimurium and Escherichia coli. In Microbiology-1984; Leive, L., Schlessinger, D., Eds.; ASM: Washington, DC, USA, 1984; p. 17.
- Gilvarg, C.; Katchalski, E. Peptide utilization in Escherichia coli. J. Biol. Chem 1965, 240, 3093–3098.
- Gallagher, M.; Pearce, S.; Higgins, C. Identification and localization of the membrane-associated, ATP-binding subunit of the oligopeptide permease of Salmonella typhimurium. Eur. J. Biochem 1989, 180, 133–141.
- Higgins, C.F.; Hiles, I.D.; Salmond, G.P.C.; Gill, D.R.; Downie, J.A.; Evans, I.J.; Holland, I.B.; Gray, L.; Buckel, S.D.; Bell, A.W.; Hermodson, M.A. A family of related ATP-binding subunits coupled to many distinct biological processes in bacteria. Nature 1986, 323, 448–450.
- Cowell, J.L. Energetics of glycylglycine transport in Escherichia coli. J. Bacteriol 1974, 120, 139–146.
- Higgins, C.F.; Hiles, I.D.; Whalley, K.; Jamieson, D.J. Nucleotide binding by membrane components of bacterial periplasmic binding protein-dependent transport systems. EMBO J 1985, 4, 1033–1039.
- Payne, J.W.; Marshall, N.J. Peptide transport. In Microbial transport systems; Winkelmann, G., Ed.; Wiley-VCH Verlag GmbH & Co. KGaA: Weinheim, Germany, 2002; p. 139.
- Mimmack, M.L.; Gallagher, M.P.; Pearce, S.R.; Hyde, S.C.; Booth, I.R.; Higgins, C.F. Energy coupling to periplasmic binding protein-dependent transport systems: stoichiometry of ATP hydrolysis during transport in vivo. PNAS 1989, 86, 8257–8261.
- Steiner, H.; Naider, F.; Becker, J.M. The PTR family: a new group of peptide transporters. Mol. Microbiol 1995, 16, 825–834.
- Gavin, J.J. Analytical microbiology: III. Turbidimetric methods. Appl. Environ. Microbiol 1957, 5, 235–243.
- Neidhardt, F.C.; Ingraham, J.L.; Schaechter, M. Growth of cells and populations. In Physiology of the bacterial cells: a molecular approach; Neidhardt, F.C., Ingraham, J.L., Schaechter, M., Eds.; Sinauer Associates: Sunderland, UK, 1990; p. 197.
- Fontaine, J. Amino acid analysis of feeds. In Amino acids in animal nutrition; D’Mello, J.P.F., Ed.; CABI Publishing: Wallingford, CT, USA, 2003; p. 15.
- Verstegen, M.W.A.; Jongbloed, A.W. Crystalline amino acids and nitrogen emission. In Amino acids in animal nutrition; D’Mello, J.P.F., Ed.; CABI Publishing: Wallingford, UK, 2003; p. 449.
- Shimomura, O.; Johnson, F.H.; Saiga, Y. Extraction, purification and properties of aequorin, a bioluminescent protein from the Luminous Hydromedusan, Aequorea. J. Cell. Comp. Physiol 1962, 59, 223–239.
- Chalfie, M.; Tu, Y.; Euskirchen, G.; Ward, W.W.; Prasher, D.C. Green fluorescent protein as a marker for gene expression. Science 1994, 263, 802–805.
- Chalova, V.; Woodward, C.L.; Ricke, S.C. Application of an Escherichia coli green fluorescent protein – based biosensor under nonsterile conditions and autofluorescence background. Lett. Appl. Microbiol 2006, 42, 265–270.
- Payne, J.W.; Gilvarg, C. Size restriction on peptide utilization in Escherichia coli. J. Biol. Chem 1968, 243, 6291–6299.
- Erickson, A.M.; Li, X.; Woodward, C.L.; Ricke, S.C. Optimisation of enzyme treatment for the degradation of feed proteins for an Escherichia coli auxotroph lysine availability assay. J. Sci. Food Agric 1999, 79, 1929–1935.
- Chalova, V.I.; Kim, W.K.; Woodward, C.L.; Ricke, S.C. Quantification of total and bioavailable lysine in feed protein sources by a whole-cell green fluorescent protein growth-based Escherichia coli biosensor. Appl. Microbiol. Biotechnol 2007, 76, 91–99.
- Chalova, V.I.; Zabala-Díaz, I.B.; Woodward, C.L.; Ricke, S.C. Development of a whole cell green fluorescent sensor for lysine quantification. World J. Microbiol. Biotechnol 2008, 24, 353–359.
- Froelich, C.A.; Ricke, S.C. Rapid bacterial-based bioassays for quantifying methionine bioavailability in animal feeds: a review. J. Rapid Methods Auto. Micro 2005, 13, 1–10.
- Zabala-Díaz, I.B.; Froelich, C.A.; Ricke, S.C. Adaptation of a methionine auxotroph Escherichia coli growth assay to microtiter plates for quantitating methionine. J. Rapid Methods Auto. Micro 2003, 10, 217–229.
- Hitchins, A.D.; McDonough, F.E.; Wells, P.A. The use of Escherichia coli mutants to measure the bioavailability of essential amino acids in foods. Plant Foods Hum. Nutr 1989, 39, 109–120.
- Tuffnell, J.M.; Payne, J.W. A colorimetric enzyme assay using Escherichia coli to determine nutritionally available lysine in biological materials. J. Appl. Bact 1985, 58, 333–341.
- Li, X.; Erickson, A.M.; Ricke, S.C. Agitation during incubation reduces the time required for a lysine microbiological growth assay using an Escherichia coli auxotrophic mutant. J. Rapid Methods Auto. Micro 2000, 8, 83–94.
- Lewis, A.J.; Bayley, H.S. Amino acid bioavailability. In Bioavailability of nutrients for animals: amino acids, minerals, and vitamins; Lewis, A.J., Ed.; Academic Press: San Diego, CA, USA, 1995; p. 35.
- D’Mello, J.P.F. Response of growing poultry to amino acids. In Amino acids in animal nutrition; D’Mello, J.P.F., Ed.; CABI Publishing: Wallingford, Connecticut, USA, 2003; p. 237.
- Krapf, G.; Bode, W. A microbiological assay based on ampicillin-induced lysis of Escherichia coli auxotrophs. Zbl. Bakt. Mik. Hyg. I. C 1980, 1, 314–319.
- Erickson, A.M.; Diaz, I.B.Z.; Kwon, Y.M.; Ricke, S.C. A bioluminescent Escherichia coli auxotroph for use in an in vitro lysine availability assay. J. Microbiol. Meth 2000, 40, 207–212.
- Li, X.; Ricke, S.C. Generation of an Escherichia coli lysA targeted deletion mutant by double cross-over recombination for potential use in a bacterial growth-based lysine assay. Lett. Appl. Microbiol 2003, 37, 458–462.
|Table 1. Assay microorganisms for amino acid quantification. OD refers to optical density.|
|Assay microorganism||Amino acid assayed||Assay response||Detection method||Reference|
|Streptococcus faecalis||Valine, Leucine|
|OD Titration||Blackmore and Parry |
Cardinal and Hedrick 
|Streptococcus zymogenes||Tryptophan, Methionine||Cell growth||OD||Wells et al. |
|Leuconostoc mesenteroides||Methionine Lysine, Arginine, Proline, Phehylalanine, Methionine, Cystine, Serine, Alanine, Aspartic acid||Cell growth|
|Blackmore and Parry |
Cardinal and Hedrick 
|Lactobacillus arabinosus||Leucine, Isoleucine, Valine, Glutamic acid||Acid production||Titration||Cardinal and Hedrick |
|Pediococcus acidilactici||Lysine, Methionine||Cell growth|
|Odunfa et al. |
|Tetrahymena pyriformis||Lysine||Cell growth||Cell count||Stott and Smith ;|
Bos et al. 
|Escherichia coli||Cysteine, Glutamine, Methionine, Lysine, Threonine, Tryptophan||Variable||Variable||Table 2 this review|
|Table 2. E. coli strains for bioavailable amino acid quantification. OD refers optical density, GFP denotes green fluorescent protein.|
|E. coli strain||Amino acid analyzed||Assay response||Detection type||Reference|
|E. coli DM 800||l - Cysteine||β-galactosidase||β-galactosidase activity||Hitchins et al. |
|E. coli M 5004 (trpA− gln−)||l - Glutamine||Cell lyses||OD||Krapf and Bode |
|E. coli ATCC 23798 (thi−)||l – Methionine||Cell growth||OD|
|Froelich et al. |
|E. coli M-26-26||l – Lysine||Cell growth||OD||Payne et al. |
|E. coli M 2626||l – Lysine||β-galactosidase||β-galactosidase activity||Tuffnell and Payne |
|E. coli CBK 140 (lysA::Tn5)||l – Lysine||β-galactosidase||β-galactosidase activity||Hitchins et al. |
|E. coli ATCC 23812 (lys−)||l – Lysine||Cell growth||Bioluminescence||Erickson et al. |
|E. coli ΔlysA (lysA−)||l – Lysine||Cell growth||OD||Li and Ricke |
|E. coli ΔlysA mini-Tn5-Km-gfpmut3||l – Lysine||Cell growth||OD; GFP fluorescence||Chalova et al. [113,114]|
|E. coli GUC 41 (metC−, thr−)||l – Methionine|
l – Threonine
|β-galactosidase||β-galactosidase activity||Hitchins et al. |
|E. coli MD 33 trpEA2−||l –Tryptophan||β-galactosidase||β-galactosidase activity||Hitchins et al. |
|Table 3. Comparison between lysine assimilation by small intestine and E. Coli.|
|Features||Small intestine||E. coli|
|Amino Acid transport||Mechanism||Passive diffusion, facilitated diffusion, active transport Active: energized by Na+-membrane gradient||Passive diffusion, facilitated diffusion, active transport Active: energized by H+-membrane gradient (lysP) and ATP-hydrolysis (LAO system)|
|Stereospecificity||Only l-amino acids are transported||Only l-amino acids are transported|
|Peptide Transport||Transporters||Distinct from amino acid transporters||Distinct from amino acid transporters|
|Peptide size||Di- and three-peptides||Di- and three-peptides|
|Stereospecificity||Peptides consist of l-amino acids||Peptides consist of l-amino acids|
|N- and C-terminal groups||Required for transport||Required for transport|
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