- freely available
Int. J. Mol. Sci. 2013, 14(10), 21167-21188; doi:10.3390/ijms141021167
Abstract: The composition of fatty acids in the diets of both human and domestic animal species can regulate inflammation through the biosynthesis of potent lipid mediators. The substrates for lipid mediator biosynthesis are derived primarily from membrane phospholipids and reflect dietary fatty acid intake. Inflammation can be exacerbated with intake of certain dietary fatty acids, such as some ω-6 polyunsaturated fatty acids (PUFA), and subsequent incorporation into membrane phospholipids. Inflammation, however, can be resolved with ingestion of other fatty acids, such as ω-3 PUFA. The influence of dietary PUFA on phospholipid composition is influenced by factors that control phospholipid biosynthesis within cellular membranes, such as preferential incorporation of some fatty acids, competition between newly ingested PUFA and fatty acids released from stores such as adipose, and the impacts of carbohydrate metabolism and physiological state. The objective of this review is to explain these factors as potential obstacles to manipulating PUFA composition of tissue phospholipids by specific dietary fatty acids. A better understanding of the factors that influence how dietary fatty acids can be incorporated into phospholipids may lead to nutritional intervention strategies that optimize health.
Dietary fatty acids can control the incidence and severity of inflammation in some diseases of humans and domestic animals. Current evidence suggests that the dietary ω-6 (n-6) to ω-3 (n-3) polyunsaturated fatty acid (PUFA) ratio is directly associated with inflammatory-based pathology in human diseases such as cancer, rheumatoid arthritis, atherosclerosis, and obesity [1–3]. Studies in production animals used for human food also suggest that dietary intake of certain PUFA can impact inflammatory responses to common infectious diseases such as mastitis and metritis [4,5]. Associations between dietary fatty acids and diseases are partially explained by the incorporation of dietary n-6 and n-3 PUFA into membrane phospholipids . The PUFA content of phospholipids influence inflammation through several mechanisms including membrane fluidity, lipid raft formation, and receptor function [7,8], but the focus of this review is on the biosynthesis of potent phospholipid-derived lipid mediators that have pro- or anti-inflammatory functions. For example, many lipid mediators produced from n-6 PUFA have pro-inflammatory functions and the overexpression of these lipid mediators is associated with the pathogenesis of inflammation during disease. Conversely, lipid mediators derived from n-3 PUFA have inflammation-resolving properties, and partly explain the disease-protective effects that are sometimes seen with n-3 PUFA ingestion . Inconsistent health benefits seen with n-3 PUFA supplementation could be due to the regulation of dietary and stored PUFA incorporation into phospholipids. Digestion, for example, can change the profile of ingested fatty acids by reducing the number of double carbon bonds [10,11]. Additionally, fatty acid incorporation into phospholipids is sometimes selective . Also, phospholipid synthetic pathways are regulated at multiple levels and are sometimes controlled by other nutrients or metabolites, such as diacylglycerol and glucose [13,14]. The objectives of this review are to explain how dietary n-6 and n-3 PUFA are incorporated into membrane phospholipids, explain how the subsequent biosynthesis of lipid mediators can influence inflammatory responses, and describe factors confounding the influence of dietary PUFA on phospholipid composition. Future studies of these confounding factors will improve knowledge of phospholipid biosynthesis in humans and domestic animals and will reveal all health outcomes of n-3 PUFA dietary supplements.
2. Trends in Dietary Fatty Acid Composition
The consumption of n-3 and n-6 PUFA in Western diets changed considerably over the last several decades . The n-6 PUFA content of Western human diets increased to some extent because plants or plant-derivatives, such as corn oil, are popular dietary ingredients . In contrast to modern Western human diets, Northern (e.g., Greenland) and Eastern (e.g., Southeast Asian) diets contain more n-3 PUFA because proportionally more dietary fatty acid is derived from fish . Marine plants and fish are rich in n-3 PUFA, relative to terrestrial plant- or animal-derived foodstuffs that are abundant in Western diets. Hence the dietary n-6 to n-3 PUFA ratio is higher in modern Western human diets compared to regions where fish remain a significant source of PUFA.
In spite of these differences in PUFA intake between regions, both n-6 and n-3 remain important dietary ingredients in all human and domestic animals. Linoleic acid (LA, C18:2 n-6) nutritional deficiency results in disease of multiple systems, including skin  and α-linolenic acid (ALA, C18:3 n-3) deficiency results in neurological impairment . These PUFA cannot be synthesized de novo but, once absorbed, they can be converted to other PUFA within the same omega designation . Domestic animals and humans cannot synthesize n-3 PUFA from n-6 because they lack specific desaturase enzymes, such as that transcribed from fat-1 in lower order eukaryotes . Therefore, the n-6 to n-3 PUFA ratio in tissue phospholipids is a direct reflection of dietary composition, although the profiles of individual n-6 and n-3 PUFA are also subject to de novo elongation and desaturation .
Like humans, many species of domestic animals have experienced significant dietary change over the past several decades. This is partly due to industrialization of Western agriculture, which reduced or eliminated pasture feeding and introduced concentrated-nutrient forages into the diet of many species, including ruminants. Meat and milk derived from intensively-raised ruminants may be partly responsible for elevated n-6 to n-3 PUFA ratios in Western human diets  as modern ruminant diets were shown to affect the n-6 to n-3 PUFA ratio of meat  and milk  from these animals. As with humans, there is increased disease risk in ruminants fed these modern diets , which can be partly explained by the n-6 to n-3 PUFA ratio in phospholipids and the effect this has on severity and duration of host inflammatory responses .
3. Dietary Polyunsaturated Fatty Acids and Inflammation
Inflammation is an essential component of the innate immune response to tissue injury. Movement of serum proteins, lipids, and blood leukocytes into affected tissues eliminate or neutralize the source of tissue injury then restore normal tissue structure and function. Failure to control the magnitude and duration of the inflammatory response can cause damage to host tissues and contribute to pathology, independent of the original insult. The ratio of n-6 to n-3 PUFA in the diet has long been recognized as an important influence on the pathogenesis of inflammation because PUFA derivatives can initiate and exacerbate inflammatory responses . This was demonstrated in several human and animal diseases, including atherosclerosis, sepsis, mastitis, and cancer [3,4,25], and involves derivatives of n-6 PUFA. In contrast, human diseases with inflammatory-based pathology were prevented with n-3 PUFA dietary supplementation. Increased fish-derived n-3 PUFA consumption, for example, was shown to lower risk of cardiovascular diseases and improved survival from myocardial infarction [26–28]. Evidence also exists that dietary n-3 PUFA dietary supplementation can prevent several forms of cancer . The inflammatory response of healthy human subjects is also affected by n-3 PUFA ingestion. For example, human mononuclear leukocytes from subjects supplemented with dietary fish-oil have decreased TNF-α expression relative to subjects consuming control diets . Despite this evidence, there remains some controversy concerning the health benefits of n-3 PUFA ingestion because not all data were conclusive. Dietary supplementation with 1 g of n-3 PUFA daily, for example, did not reduce the rate of adverse cardiovascular events in patients that had or were at risk of type 2 diabetes . Also a recent meta-study found no association between n-3 PUFA intake and incidence of major cardiovascular disease . A better understanding of how dietary PUFA are integrated into membrane phospholipids and therefore available for biosynthesis of pro-resolving mediators of inflammation may explain these equivocal results.
3.1. Phospholipids of Inflammatory Cells
The link between dietary PUFA, inflammation, and disease susceptibility is partially due to changes in the PUFA content of phospholipids in cells involved in the inflammatory response, such as monocytes, macrophages, and vascular endothelial cells [33,34]. Phospholipids are composed of 2 fatty acids esterified to glycerol at sn-1 and sn-2 and a phosphorylated head group esterified at sn-3 (Figure 1). The n-6 and n-3 PUFA, including arachidonic acid (AA, C20:4 n-6), LA, eicosapentaenoic acid (EPA, C20:5 n-3) and docosahexaenoic acid (DHA, C22:6 n-3) are incorporated into the sn-2 position of phospholipids in cellular membranes . Phospholipid head groups are cytidine-monophosphate, hydroxyl, choline, ethanolamine, serine, or inositols . Phosphocholine and phosphoethanolamine are concentrated in macrophage plasma membranes , are the major phospholipids in human plasma (76% phosphocholine and 17% phosphoethanolamine) , and are also the most abundant phospholipids in human erythrocytes . As such, phosphocholine and phosphoethanolamine are the largest phospholipid reservoirs of dietary n-6 and n-3 PUFA in cells and fluids involved in inflammatory responses.
Other less abundant phospholipids can affect inflammatory responses, but independent of lipid mediator production. For example, diphosphoglycerol (cardiolipin) consists of 2 molecules of phosphatidic acid esterified to glycerol, is the most abundant phospholipid in the inner mitochondrial membrane , and can compromise cellular respiration  and mediate apoptosis  under conditions of oxidative stress. Another example is platelet activating factor (1-O-alkyl-2-acetyl-sn-glycero-3-phosphocholine), which directly enhances cytokine and adhesion molecules expression in vascular endothelium . These are important effects of phospholipids but the objective here is to explain how major phospholipids in cells and fluids that are critical in inflammatory processes are influenced by dietary PUFA and regulate inflammatory processes when PUFAs are converted to lipid mediators of inflammation.
3.2. Inflammatory Pathways Influenced by Fatty Acid Components of Phospholipids
The fatty acid composition of membrane phospholipids in macrophages and endothelium can influence inflammatory responses in several different ways. Physical properties of membranes, such as fluidity and lipid raft formation, are influenced by specific fatty acids in membrane phospholipids and modify membrane-generated signaling cascades. For example, murine macrophage and adipocyte and human vascular endothelial cell culture studies, including some with transgenic mice, demonstrated that saturated fatty acids can directly activate proinflammatory signaling pathways through Toll-like receptor (TLR)-mediated mechanisms [42–44]. Saturated fatty acids increase proinflammatory gene expression in macrophages by inducing the dimerization and recruitment of TLR4-related signaling proteins into lipid rafts in a way that mimics endotoxin [42,45]. These responses to saturated fatty acids in phospholipids involve downstream pro-inflammatory signaling pathways. For example, treatment of murine macrophage cell lines with palmitic (C16:0) and lauric (C12:0) acids increased phosphorylation of JNK and ERK, resulting in enhanced expression of proinflammatory cytokines . Interestingly, the saturated fatty acid-induced increase in phosphorylation of MAPK signaling subunits was attenuated by increasing the DHA content of cells . This effect may be partially attributable to the direct action of n-3 PUFA and independent of conversion to lipid mediators [46,47]. Although saturated fatty acids and PUFA have important direct effects on health, the focus of this review is on conversion of n-3 and n-6 PUFA, derived from membrane phospholipids, into the more potent lipid mediators .
3.3. Phospholipid-Dependent Biosynthesis of Lipid Mediators
Several hundred lipid mediators have been identified and they collectively regulate the initiation, magnitude and duration of inflammatory responses . Eicosanoids are the most widely studied class of lipid mediators. These are derived from AA and include hydroperoxyeicosatetraenoic acids (HPETE), prostaglandins (PG), thromboxanes (TX), leukotrienes (LT), and lipoxins. The first step in eicosanoid biosynthesis occurs when esterified AA is released from membrane phospholipids by phospholipase enzymes. Intracellular AA may then be metabolized by the cyclooxygenase (COX), lipoxygenase (LOX), or epoxygenase (e.g., cytochrome P450) enzymatic pathways, which ultimately determine the class of eicosanoid generated (Figure 2). Two isoforms of COX enzymes, denoted as COX1 and COX2, are involved in the enzymatic oxidation pathways. Both COX isoforms first catalyze the oxidation of AA to prostaglandin G2 (PGG2) followed by a peroxidase reaction that reduces PGG2 to PGH2. From PGH2, specific downstream PG synthases produce PGE2, PGD2, PGI2 and PGF2α. Alternatively, thromboxane synthases convert PGH2 to TXA2 and TXB2. Similar to the COX family, there are several isoforms of LOX involved in the enzymatic oxidation of PUFA. For example, 5-LOX catalyzes the oxidation of AA to 5-HPETE that can be further metabolized to produce leukotrienes (LT). Moreover, both 15-LOX1 and 15-LOX2 oxidize AA to 15-HPETE . This can be further metabolized to lipoxin A4 by 5-LOX . The eicosanoid class of lipid mediators is predominantly proinflammatory, with a small number of exceptions. For example, lipoxin A4 is pro-resolving  and PGE2 has both proinflammatory and resolving effects . Whereas AA is the common precursor of the eicosanoid class of lipid mediators, there are other important mediators produced from the enzymatic oxidation of LA, DHA, and EPA. For example, LA is metabolized by several enzymes including 15-LOX, COX2, and the epoxygenases into hydroperoxyoctadecadienoic acid (HPODE). This is reduced to hydroxyoctadecadienoic acid (HODE), which is dehydrogenated to form oxooctadecadienoic acid (OxoODE) . The effects of LA derived mediators can be either proor anti-inflammatory [53–55]. Lipid mediators derived from n-3 PUFA are the most recently discovered . These mediators are synthesized from DHA by 12-LOX or 15-LOX and are referred to as resolvins, protectins, and maresin. In contrast to the mediators derived from n-6 PUFA, the function of mediators derived from n-3 PUFA are primarily anti-inflammatory or pro-resolving . COX2 also synthesizes resolvins from EPA, but only in patients treated with aspirin (Figure 2). Alternatively, these EPA derived resolvins can be synthesized by epoxygenases .
Enzymatic biosynthesis of lipid mediators is important because enzymes can be overexpressed in diseases such as atherosclerosis and sepsis [46,56]. Both n-6 and n-3 PUFA, however, may also undergo non-enzymatic oxidation with reactive oxygen species, resulting in production of lipid mediators with similar biological effects to those derived from enzymatic oxygenation . For example, some 15-HPETE and 13-HPODE isomers produced by non-enzymatic oxidation are identical to those synthesized by enzymatic oxidation [58,59]. These hydroperoxides are themselves reactive oxygen species, thus creating positive feedback loops on PUFA oxidation during an inflammatory response that can exacerbate disease pathogenesis.
3.4. Dietary PUFA Influence Inflammation through Lipid Mediators
There is strong evidence that the dietary n-6 to n-3 PUFA ratio influences the profile of lipid mediators within tissue [9,60,61]. For example, a recent human study demonstrated increased plasma HODE and OxoODE with increased dietary LA . Dietary supplementation with AA increased mononuclear leukocyte secretion of pro-inflammatory eicosanoids, including LTB4. EPA and DHA dietary supplementation were shown to increase lipoxins and E and D series resolvins in mouse tissue, while also decreasing pro-inflammatory AA-derived eicosanoids . Therefore in vivo production of lipid mediators is regulated by substrate availability. Some of these studies have confirmed that dietary n-6 to n-3 PUFA ratio does in fact influence lipid mediator biosynthesis through changes in PUFA composition of tissue phospholipids [9,62].
Manipulation of the profile of tissue lipid mediators by dietary PUFA is significant because lipid mediators are known to influence health. For example, increased AA-derived PGE2 biosynthesis is associated with human colon cancer [63,64]. There is increased expression of LA-derived metabolites, 9-HODE and 13-HODE, in atherosclerotic vascular lesions . Specific effects of eicosanoids on inflammation and disease pathogenesis have been demonstrated using in vivo, in vitro, and transgenic animal models of disease. For example, DHA-derived resolvin D2 was shown to ameliorate the inflammatory response in murine models of sepsis  and blockade of resolvin receptors in human polymorphonuclear leukocytes resulted in loss of the anti-inflammatory effects of resolvin D1 . PGE2 receptor deletion reduced pathology in murine models of colon cancer . Several studies showed that deletion of the 12/15-LOX gene was effective in decreasing atherosclerosis pathology in mice [68,69].
Despite cumulative evidence that changes in the profiles of eicosanoids and other lipid mediators are a major factor contributing to the health effects of PUFA intake, there are several important studies that are inconclusive. For example, a recent review of 15 human LA dietary trials found no association between intake and pro-inflammatory markers, including eicosanoids and other lipid mediators . A recent meta-analysis of the protective effects of n-3 PUFA supplementation against human cardiovascular diseases failed to identify any significant health benefits . There are several possible reasons why such inconsistency may exist in the literature. For example, lipid mediator biosynthesis is regulated at multiple levels in addition to supply of PUFA substrate. These include regulation of enzyme transcript and protein expression and enzyme activity [56,71–76]. Also, some n-6 PUFA are substrate for pro-resolving mediators, which can be displaced by n-3 PUFA supplementation . Additionally, enzymes that synthesize lipid mediators are selective in their use of substrate [77–79].
3.5. Further Lipid Mediator Research
There are some important questions that remain unanswered in this field, such as “are there potentially deleterious health effects of decreasing the tissue n-6 to n-3 PUFA ratio?” The associations between PUFA content of phospholipids and lipid mediators reveal some possible problems. For example, decreased AA-derived lipoxin-A4 biosynthesis occurs with n-3 PUFA dietary supplementation [9,80,81]. Effects such as this may not always be beneficial for health as, for example, decreased lipoxin A4 is associated with severe human asthma . The influence of DHA and EPA dietary supplements on asthmatics is not known. To address this, n-3 dietary trials should quantify all lipid mediator substrates within both diet and phospholipids of immune and vascular cells, in contrast to reporting the n-6 to n-3 PUFA ratio [83,84]. Additionally, the tissue lipid mediator profile should be assessed, in contrast to sporadic mediators in previous dietary trials [9,62]. A comprehensive profile, rather than isolated lipid mediators, is important because the lipid mediator network can function in antagonistic, synergistic, or additive manners. Having identified interactions among lipid mediators and their substrates, future research should then investigate the possible causes and interventional targets of such relationships.
Another important question is “whether n-3 PUFA supplementation ameliorates inflammation during human and animal disease because of increased biosynthesis of resolving lipid mediators from n-3 PUFA or decreased proinflammatory lipid mediator biosynthesis from n-6 PUFA?” It was reported that decreasing the tissue n-6 to n-3 PUFA ratio increases the biosynthesis of resolving type lipid mediators from n-3 PUFA and decreases the biosynthesis of proinflammatory lipid mediators from n-6 PUFA [80,81], but comparative health responses between low n-6 PUFA and high n-3 PUFA consumption are not clear. This question could be initially addressed in carefully designed dietary trials that measure phospholipid PUFA composition and lipid mediator biosynthesis of tissue.
The final question that this body of literature raises is “under which circumstances should inflammation be manipulated by dietary n-3 PUFA?” Inflammation is an essential component of mammalian physiology and exists to facilitate restoration of homeostasis in tissue. Anti-inflammatory effects of dietary PUFA may, therefore, have adverse consequences in disease recovery. This has in fact, been demonstrated with dietary n-3 PUFA supplementation in murine models of gastrointestinal inflammation . This does not imply that treatment of uncontrolled inflammation is contraindicated, but rather, that manipulation of lipid mediator biosynthesis likely has multiple outcomes and that some outcomes can be undesirable. Further evidence of this is the discovery that selective COX2 inhibitors affect vasoactive prostaglandin biosynthesis and increase risk of thromboembolic disease in humans [86,87].
4. Delivery and Utilization of Dietary PUFA for Phospholipid Biosynthesis
A better understanding of critical regulatory steps that impact phospholipid biosynthesis from dietary PUFA will provide insight into the variable success of dietary manipulation of inflammatory conditions. For example, though phospholipid biosynthesis sometimes displays a preference for absorbed PUFA, not all dietary PUFA will be used for this purpose. Also, enzymes which synthesize phospholipids are influenced by disease and physiological states, such as reproduction. Additionally, PUFA may arise at sites of phospholipid biosynthesis from body stores, such as adipose tissue, and displace dietary PUFA as substrate.
4.1. Digestion and Absorption of Dietary PUFA
PUFA are ingested in several forms, including non-esterified fatty acid, triacylglycerol, and phospholipids. Ester bonds of ingested lipids are hydrolyzed by pancreatic lipase to produce predominantly non-esterified fatty acids and monoacylglycerol . This is the primary digestive process for monogastric species, such as humans and swine and is not currently known to affect PUFA supply. However, PUFA from which lipid mediators are derived are very susceptible to non-enzymatic oxidation. For example, the anti-inflammatory effect of n-3 ingestion is increased if co-ingested with antioxidants , although it is not clear if the antioxidant effect occurs prior to n-3 absorption, or after, as demonstrated in other models . Multi-gastric species such as ruminants experience an additional digestive process which, in contrast to lipase hydrolysis, has been demonstrated to affect dietary PUFA content . This is referred to as biohydrogenation and describes hydrogenation of PUFA by the micro-flora of the fore-stomachs. Biohydrogenation reduces the efficiency of absorption of some PUFA, particularly those present in the diet at low concentrations such as EPA and DHA. For example, in vivo goat models of biohydrogenation demonstrated transfer of only 3.5% to 7.6% of dietary EPA or DHA into milk . Apparently this is sufficient to induce changes in tissue phospholipid composition, possibly because the quantity of absorbed n-3 PUFA is large relative to pre-supplementation tissue and milk levels .
The absorption process for available PUFA is similar across all domestic animal species and humans and occurs through the intestinal lymphatic system and the venous side of the vascular system . In this way, absorbed PUFA are protected from hepatic metabolism in the first pass through the circulatory system, and immediately available for biosynthesis of phospholipids in organs and cells critical in determining inflammatory responses, such as bone marrow, peripheral leukocytes, and vascular tissue [10,12].
4.2. Phospholipid Substrate from Non-Dietary PUFA
There are several important sources of non-dietary PUFA that confound the influence of dietary PUFA on inflammation (Figure 3) . These include PUFA synthesized de novo or stored in sites such as adipose tissue. The relative efficiencies of n-3 and n-6 PUFA de novo biosynthesis are controversial. For example, de novo biosynthesis of EPA and DHA from ALA has been described as modest  but there is evidence that humans have greater capacity for this than de novo biosynthesis of AA from LA . Therefore de novo biosynthesis of some n-3 PUFA cannot be discounted as having potential health benefits if this results in increased tissue content of DHA and EPA derived pro-resolving type lipid mediators.
Adipose-derived PUFA may also be used for phospholipid biosynthesis in inflammatory based cells (Figure 3). This is an abundant substrate for phospholipid synthesis during dietary restriction or large, chronic expenditures of energy because the rate of lipolysis exceeds that of lipogenesis and adipose tissue is mobilized . This occurs, for example, in humans and domestic animals during the periparturient period [94,95] because of energy expenditure associated with pregnancy and lactation and a concomitant deficit in calorie intake. During adipose mobilization, the liver can utilize adipose-derived fatty acid for ketone body biosynthesis, particularly if carbohydrate ingestion or substrates for gluconeogenesis are restricted relative to the requirements for glucose . Alternatively, fatty acid in the liver may be stored as triacylglycerol. In other organs, such as skeletal muscle, dietary and adipose-derived fatty acid can be energy substrates through β-oxidation, or in functional mammary glands, are excreted as milk lipid. Hence when adipose-derived fatty acids are mobilized into circulation, phospholipid biosynthesis must compete against ketogenesis, β-oxidation, and milk-lipid excretion for PUFA substrate. In spite of this competition, there is in vitro evidence that suggests adipose-derived fatty acids modify the composition of phospholipids in vascular endothelial tissue and induce inflammation through lipid mediators, and also evidence that this effect can be reversed with n-3 PUFA supplementation [24,74]. This is particularly interesting as there is an exacerbated inflammatory response in vivo in some species coincident with adipose mobilization . This suggests that decreasing the n-6 to n-3 PUFA ratio in adipose could potentially improve health during periods of adipose mobilization. Dietary PUFA are incorporated into adipose triacylglycerol by de novo triacylglycerol biosynthesis and remodeling through reacylation [97,98]. The rate of de novo synthesis is 20% of total triacylglycerol in healthy human adipose tissue after nine-weeks . The kinetics of triacylglycerol reacylation are not reported but since the half-life of all adipose triacylglycerol is 6-months to 2-years , it is reasonable to interpret that reacylation of adipose triacylglycerol occurs over several months or years in vivo. These data suggest that a long-term change in diet is required to induce change in adipose n-3 PUFA content. Since DHA and EPA are substrate to several inflammation-resolving lipid mediators, long-term ingestion of these, particularly during periods of triacylglycerol synthesis, could be therapeutic in inflammatory conditions associated with mobilization of adipose tissue.
Another potential origin of PUFA for phospholipids is recycled use of fatty acyl chains that have been hydrolyzed from existing phospholipids (Figure 3). Little is known about the role of this pool of fatty acids in biosynthesis of phospholipids. However, it is unlikely that the plasma membrane, the largest PUFA reservoir, has a major role in supplying PUFA for de novo phospholipids as the machinery for this are located in the endoplasmic reticulum and mitochondrion .
4.3. Effects of Disease, Physiological State, and Other Nutrients on Phospholipid Biosynthesis
De novo biosynthesis of phospholipids occurs in what is commonly referred to as the Kennedy pathway . A brief description of this pathway is useful to understand regulation of dietary PUFA incorporation into phospholipids. The first reaction in this pathway combines long-chain fatty acid with CoA and is catalyzed by acyl CoA synthase (ligase) (ACSL, Figure 4). The fatty acyl CoA is then esterified to glycerol at sn-1 on the mitochondria by glycerol-3-phosphoacyltransferase (GPAT) . The second acyltransferase is 1-acylglycerol-3-phosphoacyltransferase (AGPAT). Substrate for AGPAT is transferred from the mitochondria to the endoplasmic reticulum, and acylation occurs at sn-2 of glycerol . Glycerol esterified to fatty acid at sn-1 and sn-2 is known as phosphatidic acid. Phosphatidic acid can be metabolized by phosphatidic acid phosphatase (PPAP or lipin) to synthesize diacylglycerol. This combines with cytidine diphosphate (CDP)-choline to produce phosphocholine, which may be metabolized to phosphoethanolamine or phosphoserine. The enzyme cytidine triphosphate (CTP):phosphocholine cytidylyltransferase (CCT) catalyzes CDP-choline biosynthesis, and CDP-choline:1,2-diacylglycerol cholinephosphotransferase catalyzes the diacylglycerol reaction with CDP-choline . Triacylglycerol is the alternative diacylglycerol product, catalyzed by diacylglycerol acyltransferase (DGAT) . If phosphatidic acid is not utilized for biosynthesis of diacylglycerol, then it can be utilized by CDP-diacylglycerol synthase for synthesis of phosphoinositol, phosphoglycerol, or cardiolipin.
Expression of some phospholipid synthesizing enzymes is influenced by pathogen associated molecular patterns and so is likely influenced by bacterial infection. For example, expression of ACSL1, 3 and 4 is increased in RAW 264.7 murine macrophages in response to the TLR-4 agonist, Kdo2, an endotoxin-like molecule involved in sepsis and mastitis . Monocyte expression of ACSL1 is also increased in mouse models of type 1 diabetes, and is associated with an inflammatory phenotype and atherosclerosis . Other rodent models indicate that insulin resistance is associated with AGPAT2 and PPAP1 deficiency . The clinical relevance of these data is not currently understood but transcriptional effects suggest de novo biosynthesis of some phospholipids may change during these diseases and therefore affect how dietary PUFA are incorporated into membrane phospholipids in some patients.
Expression of some phospholipid synthesizing enzymes is also affected by physiological state. For example, ACSL1 hepatic and mammary tissue expressions are increased in dairy cattle during the postpartum period, relative to prepartum [106,107]. GPAT, AGPAT and PPAP expressions are also increased after bovine parturition [93,106,107]. Activities of some enzymes also change with physiological state. Activity of CCT, the rate limiting enzyme in phosphocholine biosynthesis, is regulated by diacylglycerol-induced intracellular translocation to membranes . Translocation results in 1.8-fold increased hepatic activity in the period immediately following parturition in cows . This may also occur when plasma and hepatic non-esterified fatty acid and di- and triacylglycerol are increased, such as in obese humans . In fact, human adipose expression of a CCT gene, Pcyt1a, is positively correlated with adipose mass . These findings indicate that the capacity for de novo biosynthesis of phospholipids may change by reproductive state and adipose mass, and warrant further investigation at all levels of enzyme regulation. Identifying certain physiological states where dietary PUFA is more successful in influencing the PUFA composition of tissue phospholipids could be used to mitigate disease risk.
Glucose has an important influence on biosynthesis of phospholipids. Glucose availability positively affects cyclin-dependent kinase cdc28, which up-regulates triacylglycerol lipase-4 activity . This results in stored fatty acids being available to phospholipids when glucose is abundant and there is a need for new membrane formation and cell proliferation. Loewen (2012) reports that glucose metabolism also influences biosynthesis of phospholipids through phosphatidic acid and the repressive transcription factor Opi1 . Specifically, under conditions of glucose starvation, intracellular pH declines and results in the release of bound Opi1 from phosphatidic acid. The released Opi1 translocates to the nucleus resulting in repression of genes involved in biosynthesis of phospholipids, and thus a conservation of stored fatty acid for more critical needs such as β-oxidation . These data indicate that phospholipid biosynthesis is affected by glucose homeostasis and suggest that dietary PUFA incorporation into phospholipids be investigated with consideration of dietary carbohydrate ingredients.
After de novo biosynthesis in the Kennedy pathway, phospholipids are continuously susceptible to post-synthetic deacylation and reacylation at the sn-1 and sn-2 fatty acyl positions (Figure 3) in what is referred to as the Lands’ cycle . This allows absorbed PUFA to quickly change the composition of tissue phospholipids, apparently within several weeks . Manipulation of PUFA in tissue phospholipids by the Lands’ cycle may be particularly successful during bacterial disease as expression of some acyltransferase enzymes is induced by TLR ligands . Further investigation of this effect may identify therapeutic applications for dietary PUFA during these diseases.
4.4. Regulation of the Acyl Composition of Phospholipid
Phospholipids have a diverse fatty acid composition. For example Quehenberger et al. (2010) measured 31 fatty-acyl variants of phosphocholine and 38 fatty-acyl variants of phosphoethanolamine in human plasma . This diversity is attributable to different combinations of long chain fatty acids at sn-1 and sn-2 of glycerol  and is determined by enzyme preference for specific fatty acid substrate. This is important because enzymes in the Kennedy pathway will define the milieu of lipid mediators produced in tissue when they show preference for substrate of lipid mediators. For example, ACSL-3 and −4 show preference for AA and EPA . AGPAT-1, prefers myristic acid (C14:0), palmitic acid, and LA-CoAs, and AGPAT-2, prefers AA-CoA . These enzymes are differentially expressed in models of sepsis and diabetes, and because of their selection of substrate, may partly explain lipid mediator biosynthesis and inflammation during these diseases [103,104]. Substrate selection by enzymes involved in tissue phospholipid biosynthesis has not been evaluated in PUFA dietary studies, but should be considered when interpreting future studies that examine the influence of dietary PUFA on lipid mediator biosynthesis.
Some Lands’ cycle enzymes are selective between fatty acids. For example, the conversion of phosphoethanolamine to phosphocholine by CDP-ethanolamine:1,2-diacylglycerol ethanolaminephosphotransferase favors biosynthesis of sn-1 palmitic acid/sn-2 DHA. This phospholipid then undergoes rapid reacylation with stearic acid (C18:0) at sn-1, and AA, LA, or DHA at sn-2. In fact, the sn-1 stearic acid/sn-2 AA forms of phosphocholine and phosphoethanolamine are usually synthesized by replacement of other acyl chains in existing phospholipids, rather than directly . Therefore the Lands’ cycle can result in rapid and preferential incorporation of DHA and other PUFA into pre-existing phospholipids. This indicates that dietary supplementation with some n-3 PUFA could have especially rapid effects on health, in light of what is known about the effect of dietary n-3 PUFA supplements on inflammation .
As mentioned previously, adipose-derived fatty acid can be a major substrate for biosynthesis of phospholipids in some physiological and disease states. In this context, selectivity of fatty acyl incorporation into triacylglycerol could affect the composition of the fatty pool available for phospholipid synthesis during mobilization of adipose. The final step in triacylglycerol synthesis involves DGAT, which adds fatty acyls to the sn-3 position of diacylglycerol. Unfortunately little research has been conducted into substrate selectivity of mammalian DGAT, but in plants it appears that DGAT-2 demonstrates preference for the less abundant, trans isomers of PUFA, and there is similar DGAT-1 and −2 specificity for palmitic acid, oleic acid (C18:1), LA, and ALA fatty acyls . In yeast, both DGAT-1 and −2 have broad substrate preferences . In reviews of these enzymes, Yen et al. (2008) suggest DGAT-1 prefers oleic over saturated fatty acyls , while others indicate DGAT-2 is required for essential fatty acyl (i.e., LA and ALA) incorporation into triacylglycerol . In summary, it appears that much work must be done before the selectivity of mammalian DGAT, and their influence on PUFA incorporation into adipose tissue, will be fully understood.
Human and animal research indicate that for dietary n-6 and n-3 PUFA to modify the pathology of disease, the PUFA content of phospholipids in cells involved in the inflammatory response must reflect the dietary PUFA composition [9,62] and specific phospholipid-derived PUFA must be utilized for biosynthesis of pro-inflammatory or pro-resolving lipid mediators . The roles of lipid mediators in maintenance of health and regulation of inflammation during disease have been introduced in the literature. Whether lipid mediators are pro-inflammatory or pro-resolving is partly determined by the specific PUFA from which the lipid mediator is derived. There are trends in the literature supporting a role for n-3 PUFA in control and prevention of inflammation during disease but it is also important to recognize that some n-6 PUFA are essential nutrients and produce pro- and anti-inflammatory lipid mediators. A number of clinical trials with patients supplemented with fish-oil showed no clear health benefit, and could be explained by factors that affect dietary PUFA incorporation into phospholipids. In conclusion, future studies of the impact of dietary PUFA on tissue phospholipid biosynthesis should examine digestive processes, competition for absorbed PUFA by other physiological processes, supply of PUFA from sources other than diet, obesity and reproductive state, glucose homeostasis, and selectivity of phospholipid synthesizing enzymes for fatty acids. Such research will improve knowledge of phospholipid biosynthesis in humans and domestic animals. Complementary studies that measure inflammatory outcomes and lipid mediator biosynthesis should reveal the true health benefit or cost of n-3 PUFA dietary supplements.
The authors acknowledge research support from the Agriculture and Food Research Initiative Competitive Grants Program (2011-67015-30179, 2012-67011-20019) from the USDA National Institute for Food and Agriculture, and an endowment from the Matilda R. Wilson Fund (Detroit, MI, USA).
Conflicts of Interest
The authors declare no conflict of interest.
- Calder, P.C. Fatty acids and inflammation: The cutting edge between food and pharma. Eur. J. Pharmacol 2011, 668, S50–S58. [Google Scholar]
- Calder, P.C.; Albers, R.; Antoine, J.M.; Blum, S.; Bourdet-Sicard, R.; Ferns, G.; Folkerts, G.; Friedmann, P.; Frost, G.; Guarner, F. Inflammatory disease processes and interactions with nutrition. Br. J. Nutr 2009, 101, 1–45. [Google Scholar]
- Simopoulos, A.P. Evolutionary aspects of diet, the ω-6/ω-3 ratio and genetic variation: Nutritional implications for chronic diseases. Biomed. Pharmacother 2006, 60, 502–507. [Google Scholar]
- Contreras, G.A.; Sordillo, L.M. Lipid mobilization and inflammatory responses during the transition period of dairy cows. Comp. Immunol. Microbiol. Infect. Dis 2011, 34, 281–289. [Google Scholar]
- Sordillo, L.M.; Contreras, G.A.; Aitken, S.L. Metabolic factors affecting the inflammatory response of periparturient dairy cows. Anim. Health Res. Rev 2009, 10, 53–63. [Google Scholar]
- Harris, W.S.; Poston, W.C.; Haddock, C.K. Tissue n-3 and n-6 fatty acids and risk for coronary heart disease events. Atherosclerosis 2007, 193, 1–10. [Google Scholar]
- Simons, K.; Toomre, D. Lipid rafts and signal transduction. Nat. Rev. Mol. Cell Biol 2000, 1, 31–39. [Google Scholar]
- Stillwell, W.; Wassall, S.R. Docosahexaenoic acid: Membrane properties of a unique fatty acid. Chem. Phys. Lipids 2003, 126, 1–27. [Google Scholar]
- Poulsen, R.C.; Gotlinger, K.H.; Serhan, C.N.; Kruger, M.C. Identification of inflammatory and proresolving lipid mediators in bone marrow and their lipidomic profiles with ovariectomy and ω-3 intake. Am. J. Hematol 2008, 83, 437–445. [Google Scholar]
- Bruss, M.L. Lipids and Ketones. In Clinical Biochemistry of Domestic Animals, 6th ed.; Kaneko, J.J., Harvey, J.W., Bruss,, M.L., Eds.; Elsevier: St. Louis, MO, USA, 2008; pp. 81–115. [Google Scholar]
- Bauman, D.E.; Harvatine, K.J.; Lock, A.L. Nutrigenomics, rumen-derived bioactive fatty acids, and the regulation of milk fat synthesis. Annu. Rev. Nutr 2011, 31, 299–319. [Google Scholar]
- Vance, D.E.; Vance, J.E. Phospholipid Biosynthesis in Eukaryotes. In Biochemistry of Lipids, Lipoproteins and Membranes, 5th ed.; Vance, D.E., Vance, J.E., Eds.; Elsevier: St. Louis, MO, USA, 2008; pp. 213–244. [Google Scholar]
- Loewen, C.J.R. Lipids as conductors in the orchestra of life. F1000 Biol. Rep 2012. [Google Scholar] [CrossRef]
- Young, B.P.; Shin, J.J.H.; Orij, R.; Chao, J.T.; Li, S.C.; Guan, X.L.; Khong, A.; Jan, E.; Wenk, M.R.; Prinz, W.A. Phosphatidic acid is a pH biosensor that links membrane biogenesis to metabolism. Sci. Signal 2010, 329, 1085–1088. [Google Scholar]
- Blasbalg, T.L.; Hibbeln, J.R.; Ramsden, C.E.; Majchrzak, S.F.; Rawlings, R.R. Changes in consumption of ω-3 and ω-6 fatty acids in the United States during the 20th century. Am. J. Clin. Nutr 2011, 93, 950–962. [Google Scholar]
- Cordain, L.; Eaton, S.B.; Sebastian, A.; Mann, N.; Lindeberg, S.; Watkins, B.A.; O’Keefe, J.H.; Brand-Miller, J. Origins and evolution of the Western diet: Health implications for the 21st century. Am. J. Clin. Nutr 2005, 81, 341–354. [Google Scholar]
- Bang, H.O.; Dyerberg, J.; Hjørne, N. The composition of food consumed by greenland eskimos. Acta Med. Scand 1976, 200, 69–73. [Google Scholar]
- Elias, P.M.; Brown, B.E.; Ziboh, V.A. The permeability barrier in essential fatty acid deficiency: Evidence for a direct role for linoleic acid in barrier function. J. Invest. Dermatol 1980, 74, 230–233. [Google Scholar]
- Delion, S.; Chalon, S.; Hérault, J.; Guilloteau, D.; Besnard, J.C.; Durand, G. Chronic dietary α-linolenic acid deficiency alters dopaminergic and serotoninergic neurotransmission in rats. J. Nutr 1994, 124, 2466–2476. [Google Scholar]
- Guillou, H.; Zadravec, D.; Martin, P.G.P.; Jacobsson, A. The key roles of elongases and desaturases in mammalian fatty acid metabolism: Insights from transgenic mice. Prog. Lipid Res 2010, 49, 186–199. [Google Scholar]
- Rule, D.C.; Broughton, K.S.; Shellito, S.M.; Maiorano, G. Comparison of muscle fatty acid profiles and cholesterol concentrations of bison, beef cattle, elk, and chicken. J. Anim. Sci 2002, 80, 1202–1211. [Google Scholar]
- White, S.L.; Bertrand, J.A.; Wade, M.R.; Washburn, S.P.; Green, J.T., Jr.; Jenkins, T.C. Comparison of fatty acid content of milk from Jersey and Holstein cows consuming pasture or a total mixed ration. J. Dairy Sci 2001, 84, 2295–2301. [Google Scholar]
- Douglas, G.; Rehage, J.; Beaulieu, A.; Bahaa, A.; Drackley, J. Prepartum nutrition alters fatty acid composition in plasma, adipose tissue, and liver lipids of periparturient dairy cows. J. Dairy Sci 2007, 90, 2941–2959. [Google Scholar]
- Contreras, G.; Mattmiller, S.; Raphael, W.; Gandy, J.; Sordillo, L. Enhanced n-3 phospholipid content reduces inflammatory responses in bovine endothelial cells. J. Dairy Sci 2012, 95, 7137–7150. [Google Scholar]
- Lawrence, T.; Gilroy, D.W. Chronic inflammation: A failure of resolution? Int. J. Exp. Pathol 2007, 88, 85–94. [Google Scholar]
- Virtanen, J.K.; Mozaffarian, D.; Chiuve, S.E.; Rimm, E.B. Fish consumption and risk of major chronic disease in men. Am. J. Clin. Nutr 2008, 88, 1618–1625. [Google Scholar]
- Galli, C.; Risé, P. Fish consumption, ω-3 fatty acids and cardiovascular disease. The science and the clinical trials. Nutr. Health 2009, 20, 11–20. [Google Scholar]
- Gruppo Italiano per lo Studio della Sopravvivenza nell’Infarto miocardico. Dietary supplementation with n-3 polyunsaturated fatty acids and vitamin E after myocardial infarction: Results of the GISSI-Prevenzione trial. Lancet 1999, 354, 447–455.
- Rose, D.P.; Connolly, J.M. Ω-3 fatty acids as cancer chemopreventive agents. Pharmacol. Ther 1999, 83, 217–244. [Google Scholar]
- Trebble, T.; Arden, N.K.; Stroud, M.A.; Wootton, S.A.; Burdge, G.C.; Miles, E.A.; Ballinger, A.B.; Thompson, R.L.; Calder, P.C. Inhibition of tumour necrosis factor-α and interleukin 6 production by mononuclear cells following dietary fish-oil supplementation in healthy men and response to antioxidant co-supplementation. Br. J. Nutr 2003, 90, 405–412. [Google Scholar]
- Bosch, J.; Gerstein, H.C.; Dagenais, G.R.; Diaz, R.; Dyal, L.; Jung, H.; Maggiono, A.P.; Probstfield, J.; Ramachandran, A.; Riddle, M.C.; et al. n-3 fatty acids and cardiovascular outcomes in patients with dysglycemia. N. Engl. J. Med 2012, 367, 309–318. [Google Scholar]
- Rizos, E.C.; Ntzani, E.E.; Bika, E.; Kostapanos, M.S.; Elisaf, M.S. Association between ω-3 fatty acid supplementation and risk of major cardiovascular disease events: A systematic review and meta-analysis. JAMA 2012, 308, 1024–1033. [Google Scholar]
- Arterburn, L.M.; Hall, E.B.; Oken, H. Distribution, interconversion, and dose response of n-3 fatty acids in humans. Am. J. Clin. Nutr 2006, 83, 1467S–1476S. [Google Scholar]
- De Mello, V.D.F.; Kolehmanien, M.; Schwab, U.; Pulkkinen, L.; Uusitupa, M. Gene expression of peripheral blood mononuclear cells as a tool in dietary intervention studies: What do we know so far? Mol. Nutr. Food Res 2012, 56, 1160–1172. [Google Scholar]
- Andreyev, A.Y.; Fahy, E.; Guan, Z.; Kelly, S.; Li, X.; McDonald, J.G.; Milne, S.; Myers, D.; Park, H.; Ryan, A.; et al. Subcellular organelle lipidomics in TLR-4-activated macrophages. J. Lipid Res 2010, 51, 2785–2797. [Google Scholar]
- Quehenberger, O.; Armando, A.M.; Brown, A.H.; Milne, S.B.; Myers, D.S.; Merrill, A.H.; Bandyopadhyay, S.; Jones, K.N.; Kelly, S.; Shaner, R.L. Lipidomics reveals a remarkable diversity of lipids in human plasma. J. Lipid Res 2010, 51, 3299–3305. [Google Scholar]
- Dowhan, W.; Bogdanov, M.; Mileykovskaya, E. Functional Roles of Lipids in Membranes. In Biochemistry of Lipids, Lipoproteins and Membranes, 5th ed.; Vance, D.E., Vance, J.E., Eds.; Elsevier: St. Louis, MO, USA, 2008; pp. 1–38. [Google Scholar]
- Paradies, G.; Petrosillo, G.; Paradies, V.; Reiter, R.J.; Ruggiero, F.M. Melatonin, cardiolipin and mitochondrial bioenergetics in health and disease. J. Pineal Res 2010, 48, 297–310. [Google Scholar]
- Musatov, A.; Robinson, N.C. Susceptibility of mitochondrial electron-transport complexes to oxidative damage. Focus on cytochrome c oxidase. Free Radic. Res 2012, 46, 1313–1326. [Google Scholar]
- Yin, H.; Zhu, M. Free radical oxidation of cardiolipin: chemical mechanisms, detection and implication in apoptosis, mitochondrial dysfunction and human diseases. Free Radic. Res 2012, 46, 959–974. [Google Scholar]
- Corl, C.; Gandy, J.; Sordillo, L. Platelet activating factor production and proinflammatory gene expression in endotoxin-challenged bovine mammary endothelial cells. J. Dairy Sci 2008, 91, 3067–3078. [Google Scholar]
- Lee, J.Y.; Sohn, K.H.; Rhee, S.H.; Hwang, D. Saturated fatty acids, but not unsaturated fatty acids, induce the expression of cyclooxygenase-2 mediated through Toll-like receptor 4. J. Biol. Chem 2001, 276, 16683–16689. [Google Scholar]
- Suganami, T.; Tanimoto-Koyama, K.; Nishida, J.; Itoh, M.; Yuan, X.; Mizuarai, S.; Kotani, H.; Yamaoka, S.; Miyake, K.; Aoe, S.; et al. Role of the Toll-like receptor 4/NF-κB pathway in saturated fatty acid-induced inflammatory changes in the interaction between adipocytes and macrophages. Arterioscler. Thromb. Vasc. Biol 2007, 27, 84–91. [Google Scholar]
- Kim, F.; Pham, M.; Luttrell, I.; Bannerman, D.D.; Tupper, J.; Thaler, J.; Hawn, T.R.; Raines, E.W.; Schwartz, M.W. Toll-like receptor-4 mediates vascular inflammation and insulin resistance in diet-induced obesity. Circ. Res 2007, 100, 1589–1596. [Google Scholar]
- Wong, S.W.; Kwon, M.J.; Choi, A.M.; Kim, H.P.; Nakahira, K.; Hwang, D.H. Fatty acids modulate Toll-like receptor 4 activation through regulation of receptor dimerization and recruitment into lipid rafts in a reactive oxygen species-dependent manner. J. Biol. Chem 2009, 284, 27384–27392. [Google Scholar]
- Li, X.; Yu, Y.; Funk, C.D. Cyclooxygenase-2 induction in macrophages is modulated by docosahexaenoic acid via interactions with free fatty acid receptor 4 (FFA4). FASEB J 2013. [Google Scholar] [CrossRef]
- Edwards, I.J.; Flaherty, J.T. Ω-3 fatty acids and PPARg in cancer. PPAR Res 2008, 2008, 358052:1–358052:14. [Google Scholar]
- Dumlao, D.S.; Buczynski, M.W.; Norris, P.C.; Harkewicz, R.; Dennis, E.A. High-throughput lipidomic analysis of fatty acid derived eicosanoids and N-acylethanolamines. Biochim. Biophys. Acta Mol. Cell Biol. Lipids 2011, 1811, 724–736. [Google Scholar]
- Dubois, R.N.; Abramson, S.B.; Crofford, L.; Gupta, R.A.; Simon, L.S.A.; van de Putte, L.B.; Lipsky, P.E. Cyclooxygenase in biology and disease. FASEB J 1998, 12, 1063–1073. [Google Scholar]
- Kuhn, H.; Thiele, B.J. The diversity of the lipoxygenase family: Many sequence data but little information on biological significance. FEBS Lett 1999, 449, 7–11. [Google Scholar]
- Serhan, C.N.; Petasis, N.A. Resolvins and protectins in inflammation resolution. Chem. Rev 2011, 111, 5922–5943. [Google Scholar]
- Calder, P.C. n-3 Polyunsaturated fatty acids, inflammation, and inflammatory diseases. Am. J. Clin. Nutr 2006, 83, S1505–S1519. [Google Scholar]
- Altmann, R.; Hausmann, M.; Spöttl, T.; Gruber, M.; Bull, A.W.; Menzel, K.; Vogl, D.; Herfarth, H.; Schölmerich, J.; Falk, W.; et al. 13-Oxo-ODE is an endogenous ligand for PPARγ in human colonic epithelial cells. Biochem. Pharmacol 2007, 74, 612–622. [Google Scholar]
- Natarajan, R.; Reddy, M.A.; Malik, K.U.; Fatima, S.; Khan, B.V. Signaling mechanisms of nuclear factor-κB-mediated activation of inflammatory genes by 13-hydroperoxyoctadecadienoic acid in cultured vascular smooth muscle cells. Arterioscler. Thromb. Vasc. Biol 2001, 21, 1408–1413. [Google Scholar]
- Ogawa, E.; Owada, Y.; Ikawa, S.; Adachi, Y.; Egawa, T.; Nemoto, K.; Suzuki, K.; Hishinuma, T.; Kawashima, H.; Kondo, H.; et al. Epidermal FABP (FABP5) regulates keratinocyte differentiation by 13(S)-HODE-mediated activation of the NF-κB signaling pathway. J. Invest. Dermatol 2011, 131, 604–612. [Google Scholar]
- Ylä-Herttuala, S.; Rosenfeld, M.E.; Parthasarathy, S.; Glass, C.K.; Sigal, E.; Witztum, J.L.; Steinberg, D. Colocalization of 15-lipoxygenase mRNA and protein with epitopes of oxidized low density lipoprotein in macrophage-rich areas of atherosclerotic lesions. Proc. Natl. Acad. Sci. USA 1990, 87, 6959–6963. [Google Scholar]
- Xu, L.; Davis, T.A.; Porter, N.A. Rate constants for peroxidation of polyunsaturated fatty acids and sterols in solution and in liposomes. J. Am. Chem. Soc 2009, 131, 13037–13044. [Google Scholar]
- Yoshida, Y.; Niki, E. Hydroxyoctadecadienoic Acid (HODE) as a Marker of Linoleic Acid Oxidation. In Biomarkers for Antioxidant Defense and Oxidative Damage: Principles and Practical Applications; Aldini, G., Yeum, K.-J., Niki, E., Russell, R.M., Eds.; Wiley: Ames, IA, USA, 2010; pp. 85–97. [Google Scholar]
- Dussault, P.; Lee, I.Q. The total synthesis of 15(S)-HPETE (hydroperoxyeicosatetraenoic acid). J. Org. Chem 1992, 57, 1952–1954. [Google Scholar]
- Ramsden, C.E.; Ringel, A.; Feldstein, A.E.; Taha, A.Y.; MacIntosh, B.A.; Hibbeln, J.R.; Majchrzak-Hong, S.F.; Faurot, K.R.; Rapoport, S.I.; Cheon, Y.; et al. Lowering dietary linoleic acid reduces bioactive oxidized linoleic acid metabolites in humans. Prostaglandins Leukot Essent. Fat. Acids 2012, 87, 135–141. [Google Scholar]
- Kelley, D.S.; Taylor, P.C.; Nelson, G.J.; Mackey, B.E. Arachidonic acid supplementation enhances synthesis of eicosanoids without suppressing immune functions in young healthy men. Lipids 1998, 33, 125–130. [Google Scholar]
- Hardardottir, I.; Kinsella, J.E. Tumor necrosis factor production by murine resident peritoneal macrophages is enhanced by dietary n-3 polyunsaturated fatty acids. Biochim. Biophys. Acta 1991, 1095, 187–195. [Google Scholar]
- Zuo, X.; Shureiqi, I. Eicosanoid profiling in colon cancer: Emergence of a pattern. Prostaglandins Lipid Mediat 2013, 104–105, 139–143. [Google Scholar]
- Wang, D.; DuBois, R.N. Prostaglandins and cancer. Gut 2006, 55, 115–122. [Google Scholar]
- Vangaveti, V.; Baune, B.T.; Kennedy, R.L. Review: Hydroxyoctadecadienoic acids: Novel regulators of macrophage differentiation and atherogenesis. Ther. Adv. Endocrinol. Metab 2010, 1, 51–60. [Google Scholar]
- Spite, M.; Norling, L.V.; Summers, L.; Yang, R.; Cooper, D.; Petasis, N.A.; Flower, R.J.; Perretti, M.; Serhan, C.N. Resolvin D2 is a potent regulator of leukocytes and controls microbial sepsis. Nature 2009, 461, 1287–1291. [Google Scholar]
- Norling, L.V.; Dalli, J.; Flower, R.J.; Serhan, C.N.; Perretti, M. Resolvin D1 limits polymorphonuclear leukocyte recruitment to inflammatory loci: Receptor-dependent actions. Arterioscler. Thromb. Vasc. Biol 2012, 32, 1970–1978. [Google Scholar]
- Rong, S.; Cao, Q.; Liu, M.; Seo, J.; Jia, L.; Boudyguina, E.; Gebre, A.K.; Colvin, P.L.; Smith, T.L.; Murphy, R.C.; et al. Macrophage 12/15 lipoxygenase expression increases plasma and hepatic lipid levels and exacerbates atherosclerosis. J. Lipid Res 2012, 53, 686–695. [Google Scholar]
- Cyrus, T.; Witztum, J.L.; Rader, D.J.; Tangirala, R.; Fazio, S.; Linton, M.; Funk, C.D. Disruption of the 12/15-lipoxygenase gene diminishes atherosclerosis in apo E-deficient mice. J. Clin. Invest 1999, 103, 1597–1604. [Google Scholar]
- Johnson, G.H.; Fritsche, K. Effect of dietary linoleic acid on markers of inflammation in healthy persons: A systematic review of randomized controlled trials. J. Acad. Nutr. Diet 2012, 112, 1029–1041. [Google Scholar]
- Gertow, K.; Nobili, E.; Folkersen, L.; Newman, J.W.; Pedersen, T.L.; Ekstrand, J.; Swedenborg, J.; Kuhn, H.; Wheelock, C.E.; Hansson, G.K.; et al. 12- and 15-lipoxygenases in human carotid atherosclerotic lesions: Associations with cerebrovascular symptoms. Atherosclerosis 2011, 215, 411–416. [Google Scholar]
- Huo, Y.; Zhao, L.; Hyman, M.C.; Shashkin, P.; Harry, B.L.; Burcin, T.; Forlow, S.B.; Stark, M.A.; Smith, D.F.; Clarke, S.; et al. Critical role of macrophage 12/15-lipoxygenase for atherosclerosis in apolipoprotein E-deficient mice. Circulation 2004, 110, 2024–2031. [Google Scholar]
- Stachowska, E.; Dziedziejko, V.; Safranow, K.; Jakubowska, K.; Olszewska, M.; Machaliñski, B.; Chlubek, D. Effect of conjugated linoleic acids on the activity and mRNA expression of 5- and 15-lipoxygenases in human macrophages. J. Agric. Food Chem 2007, 55, 5335–5342. [Google Scholar]
- Contreras, G.; Raphael, W.; Mattmiller, S.; Gandy, J.; Sordillo, L. Nonesterified fatty acids modify inflammatory response and eicosanoid biosynthesis in bovine endothelial cells. J. Dairy Sci 2012, 95, 5011–5023. [Google Scholar]
- Brinckmann, R.; Schnurr, K.; Heydeck, D.; Rosenbach, T.; Kolde, G.; Kühn, H. Membrane translocation of 15-lipoxygenase in hematopoietic cells is calcium-dependent and activates the oxygenase activity of the enzyme. Blood 1998, 91, 64–74. [Google Scholar]
- Zou, H.; Yuan, C.; Dong, L.; Sidhu, R.S.; Hong, Y.H.; Kuklev, D.V.; Smith, W.L. Human cyclooxygenase-1 activity and its responses to COX inhibitors are allosterically regulated by nonsubstrate fatty acids. J. Lipid Res 2012, 53, 1336–1347. [Google Scholar]
- Kühn, H.; Belkner, J.; Suzuki, H.; Yamamoto, S. Oxidative modification of human lipoproteins by lipoxygenases of different positional specificities. J. Lipid Res 1994, 35, 1749–1759. [Google Scholar]
- Soberman, R.; Harper, T.; Betteridge, D.; Lewis, R.; Austen, K. Characterization and separation of the arachidonic acid 5-lipoxygenase and linoleic acid ω-6 lipoxygenase (arachidonic acid 15-lipoxygenase) of human polymorphonuclear leukocytes. J. Biol. Chem 1985, 260, 4508–4515. [Google Scholar]
- Kuhn, H.; Barnett, J.; Grunberger, D.; Baecker, P.; Chow, J.; Nguyen, B.; Bursztyn-Pettegrew, H.; Chan, H.; Sigal, E. Overexpression, purification and characterization of human recombinant 15-lipoxygenase. Biochim. Biophys. Acta Lipids Lipid Metab 1993, 1169, 80–89. [Google Scholar]
- Norris, P.C.; Dennis, E.A. Ω-3 fatty acids cause dramatic changes in TLR4 and purinergic eicosanoid signaling. Proc. Natl. Acad. Sci. USA 2012, 109, 8517–8522. [Google Scholar]
- Hung, N.D.; Kim, M.R.; Sok, D.E. Oral administration of 2-docosahexaenoyl lysophosphatidylcholine displayed anti-inflammatory effects on zymosan A-induced peritonitis. Inflammation 2011, 34, 147–160. [Google Scholar]
- Levy, B.D.; Bonnans, C.; Silverman, E.S.; Palmer, L.J.; Marigowda, G.; Israel, E. Diminished lipoxin biosynthesis in severe asthma. Am. J. Respir. Crit. Care Med 2005, 172, 824–830. [Google Scholar]
- Healy, D.A.; Wallace, F.A.; Miles, E.A.; Calder, P.C.; Newsholme, P. Effect of low-to-moderate amounts of dietary fish oil on neutrophil lipid composition and function. Lipids 2000, 35, 763–768. [Google Scholar]
- Rees, D.; Miles, E.A.; Banerjee, T.; Wells, S.J.; Roynette, C.E.; Wahle, K.W.; Calder, P.C. Dose-related effects of eicosapentaenoic acid on innate immune function in healthy humans: A comparison of young and older men. Am. J. Clin. Nutr 2006, 83, 331–342. [Google Scholar]
- Woodworth, H.L.; McCaskey, S.J.; Duriancik, D.M.; Clinthorne, J.F.; Langohr, I.M.; Gardner, E.M.; Fenton, J.I. Dietary fish oil alters T lymphocyte cell populations and exacerbates disease in a mouse model of inflammatory colitis. Cancer Res 2010, 70, 7960–7969. [Google Scholar]
- Fitzgerald, G.A. Coxibs and cardiovascular disease. N. Engl. J. Med 2004, 351, 1709–1711. [Google Scholar]
- Cheng, Y.; Austin, S.C.; Rocca, B.; Koller, B.H.; Coffman, T.M.; Grosser, T.; Lawson, J.A.; FitzGerald, G.A. Role of prostacyclin in the cardiovascular response to thromboxane A2. Science 2002, 296, 539–541. [Google Scholar]
- Xiong, A.; Yu, W.; Tiwary, R.; Sanders, B.G.; Kline, K. Distinct roles of different forms of vitamin E in DHA-induced apoptosis in triple-negative breast cancer cells. Mol. Nutr. Food Res 2012, 56, 923–934. [Google Scholar]
- Kitessa, S.M.; Gulati, S.K.; Ashes, J.R.; Fleck, E.; Scott, T.W.; Nichols, P.D. Utilisation of fish oil in ruminants: II. Transfer of fish oil fatty acids into goats’ milk. Anim. Feed Sci. Technol 2001, 89, 201–208. [Google Scholar]
- Okuyama, H.; Kobayashi, T.; Watanabe, S. Dietary fatty acids—The n-6/n-3 balance and chronic elderly diseases. Excess linoleic acid and relative n-3 deficiency syndrome seen in Japan. Prog. Lipid Res 1996, 35, 409–457. [Google Scholar]
- Kris-Etherton, P.M.; Harris, W.S.; Appel, L.J. Fish consumption, fish oil, ω-3 fatty acids, and cardiovascular disease. Arterioscler. Thromb. Vasc. Biol 2003, 23, e20–e30. [Google Scholar]
- Emken, E.A.; Adlof, R.O.; Gulley, R.M. Dietary linoleic acid influences desaturation and acylation of deuterium-labeled linoleic and linolenic acids in young adult males. Biochim. Biophys. Acta BBA Lipids Lipid Metab 1994, 1213, 277–288. [Google Scholar]
- Van den Top, A.M.; Geelen, M.J.H.; Wensing, T.; Wentink, G.H.; van ’t Klooster, A.T.; Beynen, A.C. Higher postpartum hepatic triacylglycerol concentrations in dairy cows with free rather than restricted access to feed during the dry period are associated with lower activities of hepatic glycerolphosphate acyltransferase. J. Nutr 1996, 126, 76–85. [Google Scholar]
- Contreras, G.A.; O’Boyle, N.J.; Herdt, T.H.; Sordillo, L.M. Lipomobilization in periparturient dairy cows influences the composition of plasma nonesterified fatty acids and leukocyte phospholipid fatty acids. J. Dairy Sci 2010, 93, 2508–2516. [Google Scholar]
- Kaplan, A.; Lee, V.F. Serum lipid levels in infants and mothers at parturition. Clin. Chim. Acta 1965, 12, 258–263. [Google Scholar]
- Shuster, D.; Lee, E.; Kehrli, M., Jr. Bacterial growth, inflammatory cytokine production, and neutrophil recruitment during coliform mastitis in cows within ten days after calving, compared with cows at midlactation. Am. J. Vet. Res 1996, 57, 1569–1575. [Google Scholar]
- Iwasaki, Y.; Yamane, T. Enzymatic synthesis of structured lipids. Adv. Biochem. Eng. Biotechnol 2004, 90, 760–760. [Google Scholar]
- Triggiani, M.; Oriente, A.; Marone, G. Differential roles for triglyceride and phospholipid pools of arachidonic acid in human lung macrophages. J. Immunol 1994, 152, 1394–1403. [Google Scholar]
- Strawford, A.; Antelo, F.; Christiansen, M.; Hellerstein, M.K. Adipose tissue triglyceride turnover, de novo lipogenesis, and cell proliferation in humans measured with 2H2O. Am. J. Physiol. Endocrinol. Metab 2004, 286, E577–E588. [Google Scholar]
- Hodson, L.; Skeaff, C.M.; Fielding, B.A. Fatty acid composition of adipose tissue and blood in humans and its use as a biomarker of dietary intake. Prog. Lipid Res 2008, 47, 348–380. [Google Scholar]
- Kennedy, E.P.; Weiss, S.B. The function of cytidine coenzymes in the biosynthesis of phospholipides. J. Biol. Chem 1956, 222, 193–214. [Google Scholar]
- Liu, Q.; Siloto, R.M.P.; Lehner, R.; Stone, S.J.; Weselake, R.J. Acyl-CoA:diacylglycerol acyltransferase: Molecular biology, biochemistry and biotechnology. Prog. Lipid Res 2012, 51, 350–377. [Google Scholar]
- The LIPID MAPS–Nature Lipidomics Gateway. Available online: http://www.lipidmaps.org (accessed on 24 May 2012).
- Kanter, J.E.; Kramer, F.; Barnhart, S.; Averill, M.M.; Vivekanandan-Giri, A.; Vickery, T.; Li, L.O.; Becker, L.; Yuan, W.; Chait, A.; et al. Diabetes promotes an inflammatory macrophage phenotype and atherosclerosis through acyl-CoA synthetase 1. Proc. Natl. Acad. Sci. USA 2012, 109, E715–E724. [Google Scholar]
- Takeuchi, K.; Reue, K. Biochemistry, physiology, and genetics of GPAT, AGPAT, and lipin enzymes in triglyceride synthesis. Am. J. Physiol. Endocrinol. Metab 2009, 296, E1195–E1209. [Google Scholar]
- Bionaz, M.; Loor, J.J. ACSL1, AGPAT6, FABP3, LPIN1, and SLC27A6 are the most abundant isoforms in bovine mammary tissue and their expression is affected by stage of lactation. J. Nutr 2008, 138, 1019–1024. [Google Scholar]
- Loor, J.J.; Dann, H.M.; Everts, R.E.; Oliveira, R.; Green, C.A.; Guretzky, N.A.J.; Rodriguez-Zas, S.L.; Lewin, H.A.; Drackley, J.K. Temporal gene expression profiling of liver from periparturient dairy cows reveals complex adaptive mechanisms in hepatic function. Physiol. Genomics 2005, 23, 217–226. [Google Scholar]
- Bladergroen, B.A.; Wensing, T.; van Golde, L.M.G.; Geelen, M.J.H. Reversible translocation of CTP:phosphocholine cytidylyltransferase from cytosol to membranes in the adult bovine liver around parturition. Biochim. Biophys. Acta Lipids Lipid Metab 1998, 1391, 233–240. [Google Scholar]
- Xu, A.; Wang, Y.; Xu, J.Y.; Stejskal, D.; Tam, S.; Zhang, J.; Wat, N.M.S.; Wong, W.K.; Lam, K.S.L. Adipocyte fatty acid–binding protein is a plasma biomarker closely associated with obesity and metabolic syndrome. Clin. Chem 2006, 52, 405–413. [Google Scholar]
- Sharma, N.K.; Langberg, K.A.; Mondal, A.K.; Das, S.K. Phospholipid biosynthesis genes and susceptibility to obesity: Analysis of expression and polymorphisms. PLoS One 2013, 8, e65303. [Google Scholar]
- Lands, W.E. Metabolism of glycerolipides: A comparison of lecithin and triglyceride synthesis. J. Biol. Chem 1958, 231, 883–888. [Google Scholar]
- Mulligan, C.M.; Sparagna, G.C.; le, C.H.; de Mooy, A.B.; Routh, M.A.; Holmes, M.G.; Hickson-Bick, D.L.; Zarini, S.; Murphy, R.C.; Xu, F.Y.; et al. Dietary linoleate preserves cardiolipin and attenuates mitochondrial dysfunction in the failing rat heart. Cardiovasc. Res 2012, 94, 460–468. [Google Scholar]
- Shindou, H.; Hishikawa, D.; Harayama, T.; Yuki, K.; Shimizu, T. Recent progress on acyl CoA: Lysophospholipid acyltransferase research. In J. Lipid Res; 2009; Volume 50, pp. S46–S51. [Google Scholar]
- Coleman, R.A.; Lewin, T.M.; van Horn, C.G.; Gonzalez-Baró, M.R. Do long-chain acyl-CoA synthetases regulate fatty acid entry into synthetic versus degradative pathways? J. Nutr 2002, 132, 2123–2126. [Google Scholar]
- Turkish, A.; Sturley, S.L. Regulation of triglyceride metabolism. I. Eukaryotic neutral lipid synthesis: “Many ways to skin ACAT or a DGAT”. Am. J. Physiol. Gastrointest. Liver Physiol 2007, 292, G953–G957. [Google Scholar]
- Yen, C.-L.E.; Stone, S.J.; Koliwad, S.; Harris, C.; Farese, R.V. Thematic review series: Glycerolipids. DGAT enzymes and triacylglycerol biosynthesis. J. Lipid Res 2008, 49, 2283–2301. [Google Scholar]
- Zammit, V.A.; Buckett, L.K.; Turnbull, A.V.; Wure, H.; Proven, A. Diacylglycerol acyltransferases: Potential roles as pharmacological targets. Pharmacol. Ther 2008, 118, 295–302. [Google Scholar]
© 2013 by the authors; licensee MDPI, Basel, Switzerland This article is an open access article distributed under the terms and conditions of the Creative Commons Attribution license (http://creativecommons.org/licenses/by/3.0/).