Anti-mitotic effects: Growth hormone and glucocorticoids are mutually antagonistic in their effects on body growth (60) and wound healing (61), and some of the anti-mitogenic effects of glucocorticoids are mediated through changes in the hypothalamic-pituitary-liver growth hormone/IGF1 axis. Glucocorticoids disrupt the pulsatile secretory profiles of growth hormone (62,63) in rats and decrease hepatic IGF1 expression (64). They also antagonize the proliferative effects of EGF and PDGF in various cell culture systems (65,66) and antagonize the stimulatory effects of Luteinizing Hormone (LH) on the adenyl cyclase/cAMP system in Leydig cells and possibly other endocrine tissues (67,68). Although high glucocorticoid levels can cause atrophy of skeletal muscle, they stimulate hypertrophy in cardiac muscle (69). This effect is associated with alterations in expression of myosin isoforms resulting in the high efficiency V3 isoform being favored over the low efficiency V1 isoform (69,70). Thus, the anti-mitogenic effects of glucocorticoids appear to be selective.

Apoptosis plays an important role in inhibiting tumor development by eliminating damaged and genetically transformed cells from tumor susceptible tissues (71-76). Apoptosis is characterized as differing from tissue necrosis in that only selected cells are eliminated, and the resulting cell debris is immediately phagocytized by adjacent cells so that an inflammatory response is not initiated (77,78). Glucocorticoids induce apoptosis in lymphatic tissues (72), fibroblasts (79) and, possibly, in mammary epithelium (77,80). Glucocorticoids may also selectively mediate the effects of TGFß in stimulating apoptosis in preneoplastic hepatocytes (58,66).

Anti-inflammatory effects: When used therapeutically, glucocorticoids are extremely potent anti-inflammatory agents, which interact with practically every stage of the inflammatory response (81). Although it was once proposed that physiological levels of endogenous glucocorticoids stimulated the inflammatory response, as part of the general adaptation to stress (82), it now appears their physiological role during stress is to protect the organism from an overstimulated inflammatory response (81,83). Glucocorticoids achieve this by inhibiting the production of, or antagonizing the actions of, inflammatory mediators such as prostaglandins, leukotrienes, interleukins, and atrial natriuretic factor (3,21,81) [See Figure 2 following this paragraph]. Many of the anti-inflammatory and anti-mitotic effects of glucocorticoids appear to be mediated by the glucocorticoid-inducible protein, lipocortin 1 (81,84-87). Lipocortin 1 (also known as annexin 1) is a glycosylated 37 kDa Ca2+-dependent phospholipid binding protein, which inhibits phospholipase A₂, a key enzyme in the synthesis of inflammatory prostaglandins and leukotrienes from arachidonic acid (81). In addition to directly inhibiting phospholipase A₂ activity, lipocortin 1 recently has been shown to inhibit the EGF-mediated phosphorylation of the cytosolic form of this enzyme (cPLAa) (88,89). cPLAa is activated by phosphorylation as part of a G-protein dependent, EGF-mediated mitogenic response (88). Lipocortin 1 also mediates glucocorticoid feedback effects on the HPA-axis by inhibiting both basal and interleukin-induced release of CRF and AVP by the hypothalamus (55,84,90). Glucocorticoids also down-regulate mRNA expression of several key inflammatory enzymes. These include 12-lipoxygenase (91) and the inducible, but not constitutive, forms of prostaglandin synthase (COX2) (92-95), nitric oxide synthase (iNOS) (95-97) and intestinal phospholipase A₂ (PLA₂II) (98). These enzymes generally are induced by endotoxins, tumor necrosis factor, interleukins, phorbol esters, or growth factors. Although it is not known whether glucocorticoids directly or indirectly repress transcription of these enzymes, Lipocortin 1 appears to mediate glucocorticoid-mediated down-regulation of iNOS (99), but not COX2 (100).

Figure 2. Intracellular Actions of Glucocorticoids Mitogenic Signal Transduction Pathways
Glucocorticoids downregulate NF-k B and AP-1 signal transduction pathways at multiple levels. In many cell types these pathways activate inflammatory or mitogenic responses and inhibit apoptosis. In addition to transrepressing the interaction of activated NF-kB and AP-1 complexes to their DNA response elements, glucocorticoids induce proteins, which inhibit the activation of these complexes. Abbreviations used: AA = arachidonic acid, AP-1 = activator protein 1 complex (the active complex is composed of a dimer of a c-fos protein with a phosphorylated c-jun protein), cPLAa = cytosolic phospholipase A₂a, COX2 = prostaglandin synthetase (cyclooxygenase) 2, CXC = chemokines, EGF=epidermal growth factor, GC = glucocorticoid, GR = glucocorticoid receptor, GRE = glucocorticoid response element, IkB = NFk B complex inhibitor protein, Ik BK = IkB kinase, IL-1 = interleukin 1, iNOS = inducible nitric oxide synthase, JNK = Jun N-terminal kinase, LP-1 = lipocortin 1, LPS = lipopolysaccharide, LT = leukotrienes, MPK-1 = mitogen activated protein kinase phosphatase 1 (inactivates JNK by dephosphorylation), NF-kB = nuclear factor kappa B (the active complex is composed of a dimer of the P-50 and P65 proteins), PG = prostaglandins, Ps = proteasome complex which degrades phosphorylated IkB, R = plasma membrane receptors for cytokines and other inflammatory molecules, ROS = reactive oxygen species, TNFa = tumor necrosis factor alpha, TPA = 12-O-tetradecanoylphorbol-12-acetate, TRE = TPA response element.
 

Lipocortin 1 has been proposed to be a mediator of glucocorticoid-induced apoptosis. It is induced in apoptotic cells where it has been proposed to inhibit recognition of the dying cells by macrophages (77). Lipocortin 1 is also a substrate for transglutaminase. This enzyme is induced in apoptopic cells where it catalyzes the covalent linkage of proteins. Covalently linked lipocortin dimers can form polymers with other proteins during apoptosis potentially enhancing phagocytic uptake by adjacent cells (77,101,102). Lipocortin 1 was shown to protect cultured rat thymocytes from H2O2-elicited necrosis. Glucocorticoid treatment, which induced lipocortin 1, stimulated apoptosis while treatment with an anti-lipocortin 1 antibody enhanced necrosis (103).

Glucocorticoids also mediate inflammation through interactions with the nuclear factor kappa B (NF-kB) and activator protein-1 (AP-1) signal transduction pathways (104-106). Both of these pathways play a major role in the inflammatory and mitogenic responses in many cell types and in general protect cells from apoptosis when stimulated by cytokines, such as tumor necrosis factor a (TNFa) or oxidative stress (107-110). The NF-kB transcription factor complex is usually retained in the cell cytosol in an unstimulated state by an inhibitory protein (named Ik B), which binds to the cytoplasmic NF-k B complex and inhibits its translocation into the nucleus. TNFa and other cytokines stimulate the phosphorylation of IkB, which targets the inhibitor protein for proteolytic degradation, which then frees the NF-kB complex for nuclear translocation (See Figure 2 before last paragraph). Glucocorticoids induce the expression of IkB, thereby down regulating NF-kB activation, whereas insulin also stimulates IkB phosphorylation (111-114). This suggests that whether or not a cell will initiate apoptosis in response to TNFa will depend on the insulin: glucocorticoid ratio in its interstitial environment.

Activated glucocorticoid receptor complexes are also able to inhibit inflammatory and mitogenic transcription factors by direct protein-protein interaction. These interactions have been demonstrated for the NFkB complex, the AP-1 ligands c-fos and c-jun, and several STAT proteins, and are independent of glucocorticoid-mediated transcription (106,115).

Despite their global anti-inflammatory effects, glucocorticoids have been shown to potentiate certain aspects of the host defense system. For example, they have been reported to induce expression of heat shock proteins such as HSP70 (116) and increase activity of the DNA repair enzyme O6-methylguarnine-DNA methyltransferase (117) in certain tissues. They also potentiate the effects of interleukin-6 and hepatocyte-stimulating factor in inducing hepatic acute phase proteins, such as Mn-superoxide dismutase and a₂-macroglobulin (118-122). Although both glucocorticoids and lymphocyte stimulatory agents that are mediated via intracellular Ca2+ or protein kinase c (e.g., calcium ionophors/phorbol esters, antibodies to the T-cell antigen receptor) initiate apoptosis in maturing lymphocytes, they are mutually antagonistic to the extent that glucocorticoids protect lymphocytes from activation-induced apoptosis (123,124). Thus, the effects of glucocorticoids on the inflammatory and immune systems are modulatory rather than simply suppressive.

Inflammation, necrosis, oxidative damage and regenerative hyperplasia all play a significant role in chemically induced tumor promotion, and glucocorticoids have been shown to inhibit hyperplasia and neoplasia in a number of systems. For example, glucocorticoids are used therapeutically as antineoplastic agents in several types of leukemia and lymphoma (52,125), and they suppress growth of certain lung or mammary adenocarcinomas (80,126-128). Dexamethasone has been reported to inhibit both peroxisome proliferator-induced and lead nitrate-induced proliferative hyperplasia in rat liver (129,130). Glucocorticoids have also been shown to induce connexin expression and stimulate gap junction formation in cultured hepatocytes and embryonic cells (131-133). Inflammatory agents, such as phorbol esters, promote, and glucocorticoids inhibit papilloma formation in mouse skin (134).

Toxic Effects of Glucocorticoids

Chronic and excessive elevation of glucocorticoid levels increases the risk of developing hypertension, hyperkalemia, diabetes, atherosclerosis, osteoporosis, glaucoma, and impairment of the immune and reproductive systems (135,136). The organ most susceptible to glucocorticoid toxicity appears to be the hippocampus. High doses of corticosterone administered to adrenalectomized rats resulted in neuronal atrophy in the hippocampus, but not in other areas of the brain (54,137,138). Because the hippocampus, in conjunction with the hypothalamus, controls feedback regulation of the HPA, it was suggested by Sapolsky and coworkers (138), in what has become known as the glucocorticoid cascade hypothesis, that glucocorticoid-evoked hippocampal damage impairs the feedback regulation of adrenal glucocorticoid output, which could result in further increases in glucocorticoid levels and additional hippocampal damage. Over a lifetime, such an effect may result in premature aging of the brain. Evidence supporting this hypothesis includes in vitro studies, which have demonstrated that glucocorticoids impair the ability of cultured hippocampal cells to withstand neurotoxic stresses (138). The proposed mechanisms responsible for these effects include inhibition of glucose transport and disruption of Ca²⁺ homeostasis (138-140). In humans, patients with Cushing's syndrome have been reported to exhibit memory impairment, which correlated with serum cortisol levels (141), and dexamethasone treatment has been reported to impair declarative memory performance (142). However, although hypercorticism is often manifested in Alzheimer's patients (139), long-term treatment with glucocorticoids is associated with delay in the onset of Alzheimer's disease (143). Lipocortin 1 is expressed throughout the brain, including the hippocampus, and has been shown to protect against neuronal damage resulting from either ischemia or NMDA receptor agonists (144,145).

Exposure of adult rats to stress, hypercorticism or glucocorticoid therapy reduces reproductive hormone levels in both sexes (3). In males, for example, glucocorticoids appear to inhibit LH-mediated testosterone synthesis by cultured rat Leydig cells (146) and dexamethasone treatment decreases, while adrenalectomy increases serum testosterone levels  in vivo (147,148). In females, glucocorticoids decrease FSH-stimulated aromatase activity and estrogen production by ovarian granulosa cells (149), suppress ovulation and inhibit ovarian prostaglandin metabolism (150). They also inhibit the preovulatory pituitary LH surge in female rats (151) and estradiol- and gonadotropin releasing hormone-induced LH production in cultured rat pituitary cells (152). In male rats, glucocorticoids inhibit pituitary secretion of prolactin (153), but not mean LH levels (154). However, CRF and stress inhibit pituitary LH secretion in both sexes (155,156).

Glucocorticoid-Mediated Effects of Dietary Restriction

Dietary restriction not only evokes anti-inflammatory and antineoplastic effects that are consistent with chronic hypercorticism, but also protects the aging rodent against insulin resistant diabetes (29,157-159), impaired tissue growth and regeneration (160,161), certain neurological impairments (162,163), and reproductive senescence (164,165) [See Table 1 following this paragraph]. Although these latter effects appear at first sight to be inconsistent with hypercorticism, on further analysis they appear to be the natural consequence of the nutrient stress that is produced by caloric restriction under the conditions used for most experimental paradigms.

There are several factors that differentiate the nutrient stress produced by dietary restriction from other stress situations or glucocorticoid therapy (3). Firstly, unlike treatment with pharmacological doses of synthetic glucocorticoids, hypercorticism resulting from nutrient stress involves the natural glucocorticoids, corticosterone or cortisol. The effects of these natural glucocorticoids are mediated by serum transcortin and 11ß-hydroxysteroid dehydrogenase, which may protect tissues from extreme hypercorticism (3). Furthermore, unlike synthetic steroids such as dexamethasone, corticosterone and cortisol bind to both Type I and Type II glucocorticoid receptors so that the Type I receptor response is not inhibited concurrently with an excessive Type II receptor response (166).

Secondly, the hypercorticism exhibited by dietary restricted rodents differs from the continuously elevated serum corticosterone levels exhibited by starved or chronically stressed rodents in that corticosterone levels are increased, above those of their ad libitum-fed counterparts, only during a limited circadian period that is prior to and coincident with feeding activity (167). This type of intermittent hypercorticism appears to be less damaging to mitogenic processes than continuously elevated glucocorticoid levels (3).

Thirdly, because the hypercorticism is a response to caloric deficit and potential hypoglycemia and occurs in conjunction with normal feedback regulatory systems, it is not associated with chronic hyperglycemia or hyperinsulinemia (21,29,168). Thus, insulin resistance and protein glycation, which are the usual pathological consequences of glucocorticoid-induced hyperglycemia, should not occur. Instead, rates of intracellular glycation and oxidation of protein would be expected to decrease in peripheral tissues due to reduced glucose incorporation. Reduced collagen glycoxidation has been observed in skin from calorically restricted rats (169), and accumulative oxidative damage to both protein and DNA is reduced by dietary restriction in a number of tissues (59,170-176).

Fourthly, under the usual conditions that are used for dietary restriction experiments, significant hypercorticism only occurs during the early stages of restricted feeding (25,28). In most strains of rodents used in caloric restriction experiments, body weight gain is reduced in the restricted animals to an extent where the body weight difference between the restricted and  ad libitum-fed animals equals or exceeds the caloric deficit (177) [See Figure 3 following this paragraph]. Thus, during the latter half of a calorically restricted rat's life span its caloric consumption per gram body weight is equal to or greater than that of its  ad libitum-fed counterpart. Under these conditions significant hypercorticism would not be required to protect the animal from potential hypoglycemia. As a consequence, during senescence, when rodents are most susceptible to tissue degeneration due to reduced capacity for cellular proliferation and reduced output of mitogenic hormones (161,178); serum corticosterone levels are normally no longer significantly increased in chronically calorically restricted animals (3,25,28).

Figure 3. Influence of Body Weight on Caloric Consumption in Calorically Restricted Fischer 344 Rats
Fischer 344 rats, housed in a specific pathogen free barrier facility at NCTR, were placed on a vitamin fortified NIH-31 diet at 60% of ad libitum food consumption as described by Duffy et al (177). A, the weight curves for male and female rats. B, relative food consumption (expressed as food consumed per gram body weight by the calorically restricted rats as a percentage of that consumed per gram body weight by the ad libitum-fed rats) as a function of age. By 50 weeks for the males and 70 weeks for the females, the calorically restricted rats consume equivalent amounts of food per gram body weight as their ad libitum-fed counterparts.

The effects of dietary restriction on biomarkers of mitogenesis are generally consistent with the occurrence of hypercorticism during the early, but not the late stages of caloric restriction. For example, caloric restriction from 16 weeks of age abolishes growth hormone pulsatility in six month-old male Brown Norway rats, but pulsatility is restored in older animals (179). In male rats, pulsatile growth hormone controls hepatic expression of both IGF₁ and sex-specific drug metabolizing enzymes such as cytochrome P450 2C11 (CYP2C11) (180,181). As expected from its effects on pulsatile growth hormone, caloric restriction decreases hepatic expression of both IGF₁ and CYP2C11 in young male rats (182,183). However, as the rats age, hepatic IGF₁ and CYP2C11 expression decreases in the ad libitum-fed rats, but is maintained by caloric restriction animals so that in old rats hepatic IGF₁ and CYP2C11 expression is greater in the calorically restricted animals (182,183). This age-dependent biphasic effect of caloric restriction is illustrated in Figure 4 (following this paragraph) and is a common feature of several of the reported effects of caloric restriction in rodents. These include: cell proliferation rates in kidney, pancreas and possibly liver from B6D2F₁ mice (161), serum DHEA levels in Fischer 344 rats (184), and reproductive function in both rats and mice.

Figure 4. Age-dependent Effects of Caloric Restriction
(A) Schematic representation of the effects of caloric restriction on mitogenic endpoints and reproductive function. Reduction in the early burst of activity delays the degradation of these systems in old age. Examples include: [BRDU], cell proliferation in kidney tubule cells from B6D2F₁ mice, as measured by in vivo labeling with BrdU (161); [CYP] expression of hepatic cytochrome P450 2C11 (CYP2C11) and its dependent activity, testosterone 16a-hydroxylase in male Fischer 344 rats (183); [IGF] expression of hepatic IGF1 mRNA in male Fischer 344 rats (182). Caloric restriction decreases these parameters in young rats (B) but maintains them in old rats (C).

The effects of caloric restriction on female reproductive function include delayed puberty (185,186), inhibition of LH pulsatility concurrent with hypercorticism (26), inhibition of ovulation (187), decreased litter size (188,189), increased lactational diestrus (190), and reduced milk production (191) during the initial period of caloric restriction and delayed reproductive senescence during the later stage (165,188). In males, the initial effects of caloric restriction include decreased LH pulsatility (192), reduced ratios of serum testosterone to estradiol (193), decreased sperm motility in rats (194,195), and decreased prostate weight, testicular sperm density and fertility in mice (189). Long-term caloric restriction reduces testicular hyperplasia and delays Leydig cell adenoma formation in old male rats (193,196), whereas chronic feeding of a high caloric diet reduced reproductive performance in old male CF-1 mice (197).

The anti-inflammatory effects of caloric restriction are also generally consistent with effects resulting from hypercorticism. For example, caloric restriction has been reported to induce lipocortin 1 immunoreactive proteins in rat liver (21), to inhibit carrageenan-induced inflammation in mice (30), to decrease 12-lipooxygenase activity in rat liver and testes (3), to delay the onset of autoimmunity in autoimmune-prone mice (198), and to inhibit promotion of mouse skin papillomas by phorbol esters (199,200). In the last case, adrenalectomy reversed the effect of caloric restriction whereas the effect was enhanced by glucocorticoid replacement (11). Interestingly, caloric restriction both potentiates regenerative hepatocyte proliferation in partially hepatectomized rats (201) and reduces cell proliferation while stimulating apoptosis in preneoplastic liver (202,203). Such an effect is consistent with the reported dual synergistic and antagonistic effects of glucocorticoids on TGFß in neoplastic and non-neoplastic hepatocytes (3,66). Dietary restriction also reduces lung inflammation in rats exposed to ozone (204,205) and enhances resistance to gram-positive bacteria, while lowering the production of proinflammatory mediators elicited by endotoxin, a component of gram-negative bacteria.

While old dietary restricted mice exhibited improved cognitive function, motor performance, and reduced oxidative damage in the brain (162,163), dietary restriction neither inhibited hippocampal aging in rats, nor appeared to be overtly detrimental to the hippocampus (140,206). However, dieting and dietary restriction have been reported to impair cognitive function in humans (207). Despite potential endangerment to the hippocampus, hypercorticism during nutrient stress would be expected to be beneficial, since the alternative, hypoglycemia in conjunction with increased inflammatory activity, would pose a greater threat to the entire central nervous system.

Taken together, dietary restriction in rodents appears to produce a series of pleiotropic biochemical and physiological effects that are consistent with a condition hypercorticism that is more severe in the early stages of caloric restriction than in the later stages and that occurs without concurrent hyperglycemia. The overall effect of this condition is to conserve energy by minimizing metabolism, proliferation and nonessential functions in peripheral tissues. This in turn appears to minimize damage to the affected tissues so that the progression of degenerative or neoplastic lesions is delayed.

Dietary Restriction, Hypercorticism and Chemical Toxicity

Dietary restriction has been reported to increase the maximum tolerated dose or LD₅₀ of a number of chemicals (208,209) and to cause isoform-selective alterations in drug-metabolizing enzyme expression (183). While relatively large changes occur in sex-specific isoforms that are regulated by growth hormone, other isoforms are either unaffected or show moderate, circadian-dependent alterations (183). For example, 40% caloric restriction increased hepatic CYP1A-selective 7-ethoxyresorufin O-deethylase and CYP2B-selective 7-pentoxyresorufin O-dealkylase activities and immunoreactive protein in both male and female 18 week-old Fischer 344 rats, but only at specific circadian time-points (183,210). Conversely, caloric restriction decreased and eliminated the circadian variation of testicular CYP2A1-dependent testosterone 7a--hydroxylase activity (193). In addition to altering drug metabolism, it is probable that caloric restriction may also stimulate the renal clearance of drugs since caloric restriction or fasting may cause polydipsia and increase diuresis and natriuresis consistent with elevated ANP levels (177,211-213). It is possible that both these effects of fasting on serum ANP levels and of caloric restriction on polydipsia and hepatic CYP1A and CYP2B expression result from hypercorticism, since glucocorticoids induce ANP levels (214), cause polydipsia (215), and stimulate induction of CYP1A1 and CYP2B isoforms (216-218). In a recent study (219), caloric restriction was shown to enhance the induction of hepatic peroxisomal marker enzymes in B6C3F1 mice treated with chloral hydrate. This was also consistent with restriction-induced hypercorticism because glucocorticoids induce the hepatic peroxisome proliferator activated receptor PPARa.

In several cases, the effects of dietary restriction on the metabolic activation of genotoxic chemicals have been shown to correlate with specific isoform expression. For example, in vivo and  in vitro binding of aflatoxin B₁ to DNA was decreased in liver from caloric restricted rats concurrently with decreased CYP2C11, whereas binding of benzo(a)pyrene to DNA was increased concurrently with increased 7-ethoxyresorufin O-deethylase activity (183,220,221). Dietary restriction has also been reported to reduce endogenous DNA damage in liver, mammary gland and other tissues (59,170,171). However, although there are several reports demonstrating that caloric restriction increases DNA repair activity in a number of cell systems, the effect is confined mostly to old animals (222).

Dietary restriction has been shown to reduce the severity or delay the onset of carcinogenesis in rodents exposed to a number of chemical carcinogens including aflatoxin B₁, polycyclic aromatic hydrocarbons (PAH) and nitosamines (220,223-226). Although dietary restriction clearly alters the initiation stage of chemical carcinogenesis (220), it is now apparent that the major beneficial effects of caloric restriction are associated with the promotion and progression stages. This is best illustrated by experiments involving neonatal exposure of male mice to PAH (227). When mice were injected (ip) with 6-nitrochysene at 8 and 15 days post partum, they exhibited a 100% incidence liver adenomas and carcinomas when necropsied at 12 months of age. Dietary restriction (40%), initiated at 14 weeks of age, completely inhibited liver tumor formation even though the restriction was not started until after the initiation and early promotion stages of the carcinogenesis process were complete (227). Such effects are consistent with the anti-mitotic and anti-proliferative effects of caloric restriction and hypercorticism that are described above.

The observation that the body weight of rodents used in cancer bioassays directly correlates with terminal incidence of background tumors (228-231) is also consistent with effects on growth and cell proliferation, playing a major role in mediating the antineoplastic effects of caloric restriction. These body weight-tumor correlations were demonstrated from analysis of the control animals from cancer bioassays conducted by the National Toxicology Program (NTP). In B6C3F₁ mice, terminal lung tumor incidence exhibited a positive correlation with body weight at nine months on test. Conversely, terminal liver tumor incidence correlated optimally with body weight at 12 months on test (229,232). A typical correlation graph for liver tumors in male mice is shown in Figure 5 following this paragraph. In Fischer 344 rats, terminal pituitary tumor incidence exhibited a positive correlation with body weight at 13 months on test, whereas terminal leukemia incidence exhibited a positive correlation with body weight at 14 weeks (233). Interestingly, caloric restriction initiated at six weeks of age inhibited leukemia to a much greater extent than restriction initiated at 14 weeks, whereas pituitary adenoma formation was affected equally by both caloric restriction paradigms (233). This suggests that critical periods exist when rodents are most susceptible to subsequent development of specific cancer endpoints. This effect can also be demonstrated for background liver tumors in B6C3F₁ mice (231).

Figure 5. Association between Mean Body Weight and Liver Neoplasm Incidence in Male B6C3F₁ Mice
Data from control groups from nine NTP studies conducted during the 1980s and early 1990s that used water-based gavage for dosing. The percent liver neoplasm values are the survival-adjusted rates of hepatocellular adenoma or carcinoma. The individual studies used are listed in (251).

It would appear, therefore, that the rate of growth during the early adult period of an organism's life determines its subsequent susceptibility to neoplastic or degenerative diseases, and rates of growth are in part dependent on glucocorticoid status and caloric intake. Glucocorticoids are a major component of the stress and inflammatory responses, where their primary functions appear to be: [1] to globally reduce energy consumption so that energy may be channeled to the site of trauma or inflammation, and [2] to prevent excessive tissue damage due to overexpression of the inflammatory response (83). During severe nutrient stress, hypercorticism allows an organism to conserve energy so that it may survive, but in the process, growth and reproductive immune and cognitive functions may be compromised. However caloric excess may be equally detrimental resulting in overstimulated growth, uncontrolled cell proliferation, autoimmunity, inflammatory diseases, and neoplasia. Between these two extremes lies a physiological window where health and longevity is maximized. Hypercorticism, as a hormonal response to nutrient stress, appears to be common to most mammalian species and most probably evolved as a mechanism to ensure survival of the species through periods of famine (234-237). In times of abundant food supply, rapid growth and fecundity are favored over endurance and longevity. Conversely, when food becomes scarce reproductive performance and growth are sacrificed in favor of extended total and reproductive lifespans, thus increasing the probability that sufficient individuals will survive to restore the population when conditions improve. This phenomena can be observed in the human population, where rising living standards are correlated with obesity and increased cancer rates (4), as well as in rodent strains that are used in toxicology testing.

Consequences for Chronic Toxicity Testing

Over the last three decades, improvements in diet formulations and animal husbandry techniques and commercial breeding considerations have resulted in a general drift towards heavier animals for all the major rodent strains used in toxicity testing (13,14,229,230). Increase in body weight in these strains is frequently associated with decreased survival and increased susceptibility to neoplastic and degenerative diseases (13,14,165). Furthermore, interlaboratory variations in mean body weights and tumor incidence complicate comparison between studies (18).

This effect can create problems for the interpretation of chronic cancer bioassays. For example, the incidence of background liver tumors in control B6C3F₁ mice used for chronic bioassays, conducted by the NTP, has been shown to vary between 5% and 75% (238). This increased variability is partly due to altered housing conditions, but other factors such as genetic drift may also be responsible (238,239). However, differences in mean body weights between treatment groups within individual studies pose a greater problem since they may result in artifactual assumptions about the carcinogenicity of certain test chemicals (228,229).

Such differences usually arise when toxic responses to the test chemical reduce body weight gain, and a 10% reduction in body weight gain has been used as a criteria for achieving a maximum tolerated dose (240). Chemically induced body weight reductions can arise for a number of reasons, including decreased food consumption due to palatability problems in feed studies, anorexia due to toxic stress, disrupted intestinal absorption, or toxic wasting syndromes due to disruption of metabolism or endocrine systems. In most cases, such body weight gain decreases would be expected to be associated with hypercorticism, which would result from either nutrient or classic, CRF-mediated toxic stress. Nutrient stress resulting from reduced food consumption would be expected to decrease the inflammatory response in a similar manner to glucocorticoid administration or caloric restriction, whereas stress due to chemical toxicity would be expected to enhance the inflammatory response due to increased CRF and interleukin levels (See Figure 6 following this paragraph). In addition, excessive body weight gain in rodents may also involve an altered inflammatory response. Such animals could exhibit reduced efficiency in leptin expression or function, analogous to the ob/ob mouse, and this would result in hypothermia, hypercorticism, hyperglycemia, but a generally reduced inflammatory response due to elevated corticosterone (37,241,242). Conversely, they could exhibit excessive food consumption, which would result in low corticosterone levels, excessive production of arachidonic acid and an increased inflammatory response (243). Excessive inflammation exacerbates toxic responses to chemicals (244-246), directly promotes neoplasia in certain systems such as mouse skin (134) and can result in degenerative conditions such as renal inflammatory disease (243). Therefore, whether alterations in weight gain in bioassay rodents are accompanied by changes in inflammatory response may influence the relationship between body weight and terminal tumor incidence as illustrated in Figure 6 (right after this paragraph). Such effects are not only relevant to two-year cancer bioassays, but also to the ancillary studies associated with these bioassays. As noted in the previous section, diet and body weight can influence the toxicokinetics of many chemicals. Dietary restriction has also been shown to influence rates of tumor progression in transgenic mouse models that are currently being introduced for rapid carcinogenesis screens (247,248). This should be considered during the interpretation of cancer bioassay data.

Figure 6. Factors Affecting the Relationship Between Body Weight and Pathological Endpoints in Chronic Cancer Bioassays
The development of pathological lesions in rodents used in chronic bioassays is influenced by both mitogenic and inflammatory effects. Conditions, which increase inflammation in addition to increasing mitogenesis, would be expected to increase the tumor risk to a greater extent than predicted by body weight alone.

Dietary restriction has been suggested as a possible means for eliminating background tumors from the bioassay control populations (14,15). However, as stated above, dietary restriction inhibits chemically induced carcinogenesis in rodents (230,238,249). Moreover, dietary restriction is generally implemented by limiting food consumption to a set percentage of ad libitum food consumption, and this may vary between rodent populations in different laboratories (230,238).

An alternative approach involves using dietary control to manipulate the body weights and growth rates of rodents used in bioassays so that they conform to strain-specific standardized weight curves. Such standardized or idealized weight curves have been created for male and female B6C3F₁ mice and could potentially be used throughout industry and the regulatory community to standardize background neoplasm incidences between laboratories (3). The body weights of mice used for both control and treatment groups in future bioassays could be manipulated to fit these growth curves by moderate feed restriction or dietary supplementation.

Testing Dietary Control

The concept of using idealized weight curves has recently been tested as part of a standard NTP bioassay of chloral hydrate in B6C3F₁ mice that was conducted at the National Center for Toxicological Research [NCTR] (219,231,250-252). Data from mice used in NTP and NCTR chronic bioassays and aging studies were used to construct idealized weight curves for male and female B6C3F₁ mice that predicted a liver neoplasm incidence of 15% to 20% at 26 months of age. A 15% to 20% liver neoplasm incidence is sufficiently high to guarantee that the sensitivity of the mouse to chemical carcinogenesis has not been compromised, and it is low enough to ensure that the spontaneous neoplasms will not obscure any chemically induced liver tumors, and that sufficient mice will survive to the end of a two-year study. Initially the relationship between body weight and liver tumor incidence was calculated for historical control populations of male and female ad libitum-fed mice (approx. 2,750 and 2,300 animals respectively). However, it was determined that male B6C3F₁ mice, which had been subjected to forced body weight reduction due to either dietary restriction or exposure to non-carcinogenic test chemicals, differed from ad libitum-fed mice in their relationship between body weight and tumor incidence. A second weight-reduced historical control population (approx. 1,600 animals) was therefore used to construct the idealized weight curve for male mice (231). These curves are shown in Figure 7 following this paragraph.

Figure 7. Idealized Body Weight Curves for Male and Female B6C3F1 Mice
Body weights for ad libitum-fed and 40% calorically restricted mice from caloric restriction studies performed at NCTR are shown for comparison. Food consumption data from these mice were used to construct a feeding schedule used for manipulating the animals’ weights to fit the idealized body weight curve. Taken from Leakey et al. (231), full details are given in this reference.

Weight-reduced mice exhibited a more linear relationship between body weight and liver tumor incidence in the low weight range than did ad libitum-fed mice, which exhibited a J-curve profile (3,229,231). These differences did not occur in females and were less apparent in sexually senescent males older than 60 weeks (See Figure 8 following this paragraph) and result in a larger sex-difference in liver tumor incidence in light mice than in heavy mice (231).

 
Figure 8. Liver Tumor Risk Curves for Ad Libitum-fed Male and Female, and Weight-Reduced Male B6C3F₁ Mice at Various Ages
Liver tumor risk curves were constructed as described in Leakey et al (231) from body weight values corresponding to the ages shown on each graph. They are plotted as spline curves rather than bar graphs. The dotted line represents the target tumor risk (17.5%) for the idealized weight curve.

It is probable that stress due to dietary restriction or chemical exposure reduces not only the body weight-related liver tumors in male mice, but also the sex-dependent liver tumors which occur independently of body weight in small male B6C3F₁ mice and cause the J-curve profile in the tumor risk curve. Castration studies with the parent strains of B6C3F₁ mice, which also show sex differences in liver neoplasm risk, suggest that this increased incidence of liver neoplasms in the small male mice is partly due to testicular androgens (253-255). As discussed above, short-term caloric restriction has been reported to reduce the testosterone/estradiol ratios and impair male reproductive function in rodents, and restraint stress or food depression suppresses LH secretion in male mice (256).

The NCTR bioassay of chloral hydrate compared dietary-controlled mice with ad libitum-fed mice. Groups of 120 male mice received chloral hydrate in distilled water by gavage at doses of 0, 25, 50, or 100 mg/kg, 5 days per week for 104 to 105 weeks; vehicle controls received distilled water only. Each dose group was divided into two dietary groups of 60 mice. The  ad libitum-fed mice had feed (NIH-31 autoclaved pelleted diet, Purina Mills, Richmond, IN) available ad libitum, and the dietary-controlled mice received the same feed in measured daily amounts calculated to maintain body weight on a previously computed idealized body weight curve. Twelve mice from each diet/dose group were evaluated at 15 months. Weekly feed allocation values required to control body weight in mice to conform to the idealized body weight curve were calculated as grams of NIH-31 pellets per day from food consumption and body weight data from previous NCTR studies using B6C3F1 mice. This is described in detail elsewhere (231). It was anticipated that individual mice would exhibit body weights that differed significantly from the idealized body weight curve at certain times during their growth. These mice were identified on a weekly basis and their food allocation adjusted in either 1.0 or 1.5 g increments to manipulate the body weight back onto the idealized body curve.

While chloral hydrate was less potent than expected, it did produce a weak, but statistically significant, hepatocarcinogenic response in both the ad libitum-fed and the dietary-controlled mice (See Table 2 immediately following).

In the ad libitum-fed mice, this consisted of a significant increase in combined hepatocellular adenoma and carcinoma incidence in the 25-mg/kg-dose group with no further increase at higher doses. In the dietary-controlled mice, the combined hepatocellular adenoma and carcinoma incidence increased from 23.4% in the control group to 38.6% in the 100 mg/kg dose group, with a statistically significant dose trend; this increase was due to a statistically significant increase in hepatocellular carcinomas in the high dose group. Observed numbers of liver tumors were less in all the dietary-controlled dose groups than in the corresponding ad libitum-fed dose groups. Dietary control also significantly increased survival in the control, 25 and 50 mg/kg dose groups and decreased body weight variability in all groups. Dietary control reduced individual body weight variation in all four-dose groups (See Figures 9 & 10 immediately following).

Figure 9. Growth Curves for Ad Libitum-Fed and Dietary-Controlled from the Chloral Hydrate Study - Low Dose and Vehicle Control Groups
The graphs show the standard deviation of each weekly mean body weight values for the control and 25 mg/kg chloral hydrate dose groups respectively. The idealized weight curve and the NCTR historical growth curve for male B6C3F₁ mice are shown on each graph for reference. The arrow marks the time point at which 12 mice were removed for the interim evaluation.

Figure 10. Growth Curves for Ad Libitum-Fed and Dietary-Controlled from the Chloral Hydrate Study -Medium and High Dose Groups
The graphs show the standard deviation of each weekly mean body weight values for the 50 and 100 mg/kg chloral hydrate dose groups respectively. Other details are given in Figure 9.

This was associated with smaller variation in related parameters. For example, a significant dose-response in liver per body weight values was observed in dietary-controlled mice used for an interim evaluation in the study (252), whereas a significant dose response was not observed in the ad libitum-fed mice, which exhibited much greater individual variation (See Table 3 following this paragraph).

The dietary control procedures were relatively easy to run in this study and did not generate a large amount of extra labor once the feed allocation software had been developed. Access to a feed pellet sorter and prior experience with caloric restriction studies also facilitated diet preparation. Since the study used gavage dosing, weekly weights were readily available. The procedure would be potentially more expensive and complicated for studies, which dose via the feed because these animals are generally not weighed every week, and the variable amounts of feed required for dietary control would result in variable dose levels. However, dose variation occurs in all feed studies since individual animals consume different amounts of feed. Dietary control could in fact standardize dosing to a more defined level if the required level of dietary restriction is relatively high and each animal consumes its entire daily feed allowance (231, 250).

During the course of this study, a procedure was developed to use the historical control data from ad libitum-fed and weight-reduced mice to calculate predicted background liver tumor rates for individual mice based on their body weight values between 21 and 68-weeks of age. Full details of this procedure are given elsewhere (231). Using this procedure, it was possible to predict background liver tumor rates for each experimental group in the chloral hydrate study as shown in Table 4 (following this sentence)

and Figure 11 (following this paragraph), this procedure was able to accurately predict the background tumor rates in both the dietary-controlled and the ad libitum-fed dose-control groups. As illustrated in Figure 11 (following this paragraph), the variation in predicted background liver tumor risk of individual mice in each dose group was much less for the dietary-controlled mice than for the ad libitum-fed mice. Furthermore, the technique showed the observed liver tumor incidence in the dietary-controlled 50 mg/kg and 100 mg/kg dose groups were significantly greater than predicted background tumor incidence even though these groups did not show a statistically significant increase on the Poly-3 test (Table 2). This is because the Z_tr statistic used in Table 4 (above this paragraph) is an estimate of the probability that the observed tumor rate is an acceptable background tumor rate for the body weight-adjusted historical control population and is dependent on the variance of calculated tumor risk of the mice in each group rather than assuming a fixed binomial variance (231). As such it can give valuable supportive evidence on the relevance of test chemically induced increases in tumor incidence, but it assumes that no other factors significantly influence tumor incidence between studies other than body weight, survival and the test chemical.

Figure 11. Cumulative Tumor Risk Plots for the Chloral Hydrate Study
The mice from each experimental group were sorted by tumor risk into sequential 2% incremental groups. Tumor risk was calculated for the ad libitum-fed mice by sorting by body weight decrease and for the dietary controlled mice by sorting by "< 5% ad libitum" (see Table 4). Each mouse is represented in the incremental group by its a value to adjust for intercurrent mortality. The Gaussian distributions for each experimental group are calculated from the means and standard deviations of the adjusted tumor risk values given in Table 4. Taken from Leakey et al (231), full details are given in this reference.

Dietary control, therefore, can potentially improve both the sensitivity and reproducibility of cancer bioassays in mice. However, mouse liver neoplasms are frequently induced epigenetically by chemicals, which appear to not be carcinogenic for humans (257-259). Moreover, although incidence of liver cancer is increasing in the U.S. and other Western countries, the primary risk factor appears to be chronic inflammation resulting from hepatitis C or B infection rather than linked to the ongoing rise in obesity or exposure to chemical carcinogens (260-262). It could therefore be argued that a more sensitive mouse bioassay would merely compound the problem of accumulating misleading or false positive animal data that are irrelevant to human risk. Thus, it might not be useful to the regulatory community.

There are two main answers to this. First, it must be remembered that most other neoplastic lesions are also reduced by caloric restriction and related stress responses. For example, in B6C3F₁ mice positive correlations have been reported between body weight and incidence of tumors of the pituitary gland, lung and Harderian gland and of hemangiomas/hemangiosarcomas in addition to liver tumors (229,232). Caloric restriction has also been shown to delay or inhibit the development of these tumor types in B6C3F₁ mice (263). Reducing variability and body weight artifacts will therefore increase sensitivity to detect a wide range of neoplastic responses in addition to liver tumors.

Second, many potent genotoxic chemicals also cause liver tumors in B6C3F₁ mice, and several are hepatocarcinogenic in humans (264,265). Evidence as to whether a positive tumor response has relevance to humans and whether safe exposure levels can be determined depends on mechanistic data ancillary to bioassay tumor data. The emerging revolution in “-omics “ technology holds promise that such mechanistic data will become more comprehensive and informative, but it is dependent on the quality and reproducibility of available tissue samples. Microarray techniques are especially vulnerable to sample variation, because of the large number of interactive endpoints that have to be measured simultaneously. Dietary control offers an approach to greatly reduce both variability within studies and between studies.

Acknowledgments

We thank Ronald Hart, Peter Duffy and Angelo Turturro for helpful discussions; Clyde Ulmer, Barbara Hampton, Sandra Goldman, and Kathy Carrol of Northrop Grumman, NCTR, for their help in data processing; Martin Nichols, The Bionetics Corporation, NCTR, for his expertise in maintaining the mice on dietary control; and Richard Morris and Analytical Sciences Inc., Durham, N.C., for providing data from the NTP database. This work was sponsored in part by NIA-NCTR contract 224-86-001, NIEHS-NTP contract 224-933-0001 and the NCTR.

References

1. Weindruch, R. and Walford, R. (1988). Retardation of aging and disease by dietary restriction. Thomas Press, Springfield, IL.
2. Allaben, W. T., Chou, M. W., Pegrem, R. A., Leakey, J. E. A., Feuers, R. J., Duffy, P. H., Turturro, A., and Hart, R. W. (1990). Modulation of toxicity and carcinogenesis by caloric restriction. Korean J. Toxicol. 6:167-182.
3. Leakey, J. E. A., Seng, J. E., Barnas, C. R., Baker, V. M., and Hart, R. W. (1998). A mechanistic basis for the beneficial effects of dietary restriction on longevity and disease. Consequences for the interpretation of rodent toxicity studies. Intnl. J. Toxicol. 17 Suppl. 2:5-57.
4. Frame, L. T., Hart, R. W., and Leakey, J. E. A. (1998). Caloric Restriction as an Adaptive Mechanism Mediating Resistance to Environmental Disease. Environ. Hlth. Persp. 106, Suppl 1:313-324.
5. Masoro, E. J. (1998). Influence of caloric intake on aging and on the response to stressors. Journal of Toxicology & Environmental Health. Part B, Critical Reviews 1:243-257.
6. Masoro, E. J. (2001). Dietary restriction: current status. Aging (Milano) 13:261-262.
7. Hasty, P. (2001). The impact energy metabolism and genome maintenance have on longevity and senescence: lessons from yeast to mammals. Mechanisms of Ageing & Development 122:1651-1662.
8. Kritchevsky, D. (2001). Caloric restriction and cancer. Journal of Nutritional Science & Vitaminology 47:13-19.
9. Leakey, J. E. A., Harmon, J. R., Bazare, J. J., Jr., Chen, S., Manjgaladze, M., Feuers, R. J., Duffy, P. H., and Hart, R. W. (1991). Role of corticosteroids and "caloric stress" in modulating the effects of caloric restriction in rodents. Age 14:134 (Abstract)
10. Han, E. -S., Levin, N., Bengani, N., Roberts, J. L., Suh, Y., Karelus, K., and Nelson, J. F. (1995). Hyperadrenocorticism and food restriction-induced life extension in the rat: Evidence for divergent regulation of pituitary proopiomelanocortin RNA and adrenocorticotropic hormone biosynthesis. J. Gerontol. 50A:B288-B294
11. Liu, Y., Wang, W., Hawley, J., and Birt, D. F. (2002). Adrenalectomy abrogates reduction of 12-O-tetrade-canoylphorbol-13-acetate-induced extracellular signal-regulated protein kinase activity in the epidermis of dietary energy-restricted SENCAR mice: implications of glucocorticoid hormone. Cancer Epidemiology, Biomarkers & Prevention 11:299-304.
12. Tannenbaum, A. (1940). Relationship of body weight to cancer incidence. Arch. Pathol. 30:509-517.
13. Nohynek, G J., Longeart, L., Geffray, B., Provost, J. P. and Lodole, A. (1993). Fat, frail and dying young: Survival, body weight and pathology of the Charles River Sprague-Dawley-derived rat prior to and since the introduction of the VAFR variant in 1988. Human Exp. Toxicol. 12:87-98.
14. Roe, F. J. C. (1993). What does carcinogenicity mean and how should we test for it? Food Chem. Toxicol., 31:225-229.
15. Keenan, K. P., Smith, P. F., Hertzog, P., Soper, K., Ballam, G. C., and Clark, R. L. (1994). The effects of overfeeding and dietary restriction on Sprague-Dawley rat survival and early pathology biomarkers of aging. Toxicologic Pathol. 22:300-315.
16. Hart, R. W., Neumann, D. A., and Robertson, R. T. (1995). Dietary restriction. Implications for the design and interpretation of toxicity and carcinogenicity studies. ILSI Press, Washington, D.C.
17. Hart, R. W., Leakey, J., Duffy, P. H., Feuers, R. J., and Turturro, A. (1996). The effects of dietary restriction on drug testing and toxicity. Exp. Toxic. Pathol. 48:121-127.
18. Allaben, W. T., Turturro, A., Leakey, J. E. A., Seng, J. E., and Hart, R. W. (1996). Points-to-Consider Documents: The need for dietary control for the reduction of experimental variability within animal assays and The use of dietary restriction to achieve dietary control. Toxicologic Pathol. 24:776-781.
19. Greenwald, P. and Sondik, E. (1986). Diet and chemoprevention in NCI's research strategy to achieve national cancer control objectives. Ann. Rev. Public Hlth. 7:267-291.
20. Rao, G. N. (1997). New nonpurified diet (NTP-2000) for rodents in the National Toxicology Program's toxicology and carcinogenesis studies. J. Nutr. 127:842S-846S.
21. Leakey, J. E. A., Chen, S., Manjgaladze, M., Turturro, A., Duffy, P. H., Pipkin, J. L., and Hart, R. W. (1994). Role of glucocorticoids and "caloric stress" in modulating the effects of caloric restriction in rodents. Annal. N.Y. Acad. Sci. 719: 171-194.
22. Boutwell, R. K., Brush, M. K., and Rusch, H. P. (1948). Some physiological effects associated with chronic caloric restriction. Am. J. Physiol. 154:517-524.
23. Honma, K. I., Honma, S., and Hiroshige, T. (1983). Critical role of food amount for prefeeding corticosterone peak in rats. Am. J. Physiol. 245:R339-R344
24. Armario, A., Montero, J. L., and Jolin, T. (1987). Chronic food restriction and the circadian rhythms of pituitary-adrenal hormones, growth hormone and thyroid-stimulating hormone. Annal. Nutr. Metab. 31:81-87.
25. Stewart, J., Meaney, M. J., Aitken, D., Jensen, L., and Kalant, N. (1988). The effects of acute and life-long food restriction on basial and stress-induced serum corticosterone levels in young and aged rats. Endocrinology 123:1934-1941.
26. Bronson, F. H. and Heideman, P. D. (1990). Short-term hormonal responses to food intake in peripubertal female rats. Am. J. Physiol. 259:R25-R31
27. Leakey, J. E. A., Bazare, J., Jr., Harmon, J. R., Feuers, R. J., Duffy, P. H., and Hart, R. W. (1991). Effects of long-term caloric restriction on hepatic drug metabolizing enzyme activities in the Fischer 344 rat. In: Biological effects of dietary restriction, edited by L. Fishbein, pp. 207-216. Springer-Verlag, New York.
28. Sabatino, F., Masoro, E. J., McMahan, C. A., and Kuhn, R. W. (1991). Assessment of the role of the glucocorticoid system in aging processes and in the action of the food restriction. J. Gerontol. 46:B171-B179
29. Harris, S. B., Gunion, M. W., Rosenthal, M. J., and Walford, R. L. (1994). Serum glucose, glucose tolerance, corticosterone and free fatty acids during aging in energy restricted mice. Mech. Ageing Devel. 73:209-221.
30. Klebanov, S., Diais, S., Stavinoha, W. B., Suh, Y., and Nelson, J. F. (1995). Hyperadrenocortism, attenuated inflammation, and the life-prolonging action of food restriction in mice. J. Gerontol. 50A:B78-B82
31. Strack, A. M., Sebastian, R. J., Schwartz, M. W., and Dallman, M. F. (1995). Glucocorticoids and insulin: reciprocal signals for energy balance. Am. J. Physiol. 268:R142-R149
32. Dallman, M. F., Strack, A. M., Akana, S. F., Bradbury, M. J., Hanson, E. S., Scribner, K. A., and Smith, M. (1993). Feast and famine: critical role of glucocorticoids with insulin in daily energy flow. Frontiers Neuroendocrinol. 14:303-347.
33. White, B. D. and Martin, R. J. (1997). Evidence for central mechanism of obesity in the Zucker rat: Role of neuropeptide Y and leptin. Proc. Soc. Exp. Biol. Med. 214:222-232.
34. Larsen, P. J., Jessop, D. S., Chowdrey, H. S., Lightman, S. L., and Mikkelsen, J. D. (1994). Chronic administration of glucocorticoids directly upregulates prepro-neuropeptide Y and Y1-receptor mRNA levels in the arcuate nucleus of the rat. J. Neuroendocrinol. 6: 153-159.
35. Halaas, J. S., Gajiwala, K. S., Maffei, M., Cohen, S. L., Chait, B. T., Rabinowitz, D., Lallone, R. L., Burley, S. K., and Freidman, J. M. (1995). Weight-reducing effects of the plasma protein encoded by the obese gene. Nature 269:543-546.
36. MacDougald, O. A., Hwang, C.-S., Fan, H., and Lane, M. D. (1995). Regulated expression of the obese gene product (leptin) in white adipose tissue and 3T3-L1 adiposites. Proc. Natl. Acad. Sci. USA 92:9034-9037.
37. Pelleymounter, M. A., Cullen, M. J., Baker, M. B., Hecht, R., Winters, D., Boone, T., and Collins, F. (1995). Effects of the obese gene product on body weight regulation in ob/ob mice. Nature 269:540-543.
38. Saladin, R., De Vos, P., Guerre-Millo, M., Lecturque, A., Girard, J., Staels, B., and Auwerx, J. (1995). Transient increase in obese gene expression after food intake or insulin administration. Nature 377:527-529.
39. Margetic, S., Gazzola, C., Pegg, G. G., and Hill, R. A. (2002). Leptin: a review of its peripheral actions and interactions. International Journal of Obesity & Related Metabolic Disorders: Journal of the International Association for the Study of Obesity 26:1407-1433.
40. Elimam, A. and Marcus, C. (2002). Meal timing, fasting and glucocorticoids interplay in serum leptin concentrations and diurnal profile. European Journal of Endocrinology 147:181-188.
41. Suemaru, S., Hashimoto, K., Hattori, T., Inoue, H., Kageyama, J., and Ota, Z. (1986). Starvation-induced changes in rat brain corticotropin-releasing factor (CRF) and pituitary-adrenocortical response. Life Sci. 39:1161-1166.
42. Muret, L., Priou, A., Oliver, C., and Grino, M. (1992). Stimulation of adrenocorticotropin secretion by insulin-induced hypoglycemia in the developing rat involves arginine vasopressin but not corticotropin-releasing factor. Endocrinology 130:2725-2732.
43. Leal, A. M., Forsling, M. L., and Moreira, A. C. (1995). Diurnal variation of the pituitary-adrenal and AVP responses to stress in rats under food restriction. Life Sci. 56:191-198.
44. Andreis, P. G., Tortorella, C., and Nussdorfer, G. G. (1993). Pancreatic polypeptide stimulates corticosterone secretion by isolated rat adrenocortical cells. Life Sci. 53:1353-1356.
45. Mazzocchi, G., Malendowicz, L. K., Gottardo, G., Meneghelli, V., and Nussdorfer, G. G. (1995). Pancreatic polypeptide enhances plasma glucocorticoid concentration in rats: Possible role in hypoglycemic stress. Life Sci. 56:595-600.
46. Rebuffat, P., Malendowicz, L. K., Meneghelli, V., Macchi, V., and Nussdorfer, G. G. (1998). Pancreatic polypeptide stimulates rat adrenal glucocorticoid secretion by activating the adenylate cyclase-dependent signaling pathway. Life Sci. 62:1217-1222.
47. Andreis, P. G., Neri, G., and Nussdorfer, G. G. (1991). Corticotropin-releasing hormone (CRH) directly stimulates corticosterone secretion by the rat adrenal gland. Endocrinology 128:1198-1200.
48. Tsujimoto, S., Okumura, Y., Kamei, C., and Tasaka, K. (1993). Effects of intracerebroventricular injection of histamine and related compounds on corticosterone release in rats. Br. J. Pharmacol. 109:807-813.
49. Kramer, R. E., Buster, J. E., and Andersen, R. N. (1990). Differential modulation of ACTH-stimulated cortisol and androstenedione secretion by insulin. J. Steroid Biochem. 36:33-42.
50. Shafagoj, Y., Opoku, J., Qureshi, D., Regelson, W., and Kalimi, M. (1992). Dehydroepiandrosterone prevents dexamethasone-induced hypertension in rats. Am. J. Physiol. 263:E210-E213
51. Kalimi, M., Shafagoj, Y., Loria, R., Padgett, D., and Regelson, W. (1994). Anti-glucocorticoid effects of dehydroepiandrosterone (DHEA). Mol. Cell. Biochem. 131:99-104.
52. Regelson, W. and Kalimi, M. (1994). Dehydroepiandrosterone (DHEA)--the multifunctional steroid. II. Effects on the CNS, cell proliferation, metabolic and vascular, clinical and other effects. Mechanism of action? Annal. N.Y. Acad. Sci. 719:564-575.
53. Regelson, W., Loria, R., and Kalimi, M. (1994). Dehydroepiandrosterone (DHEA)--the "mother steroid". I. Immunologic action. Annal. N.Y. Acad. Sci. 719:553-563.
54. Landfield, P. W. (1987). Modulation of brain aging correlates by long-term alterations of adrenal steroids and neurally-active peptides. Prog. Brain Res. 72:279-300.
55. Buckingham, J. C., Loxley, H. D., Taylor, A. D., and Flower, R. J. (1994). Cytokines, glucocorticoids and neuroendocrine function. Pharmacol. Res. 30:35-42.
56. Debons, A F., Zurek, L. D., Tse, C. S., and Abrahamsan, S. (1986). Central nervous system control of hyperphagia in hypothalamic obesity: dependence on adrenal glucocorticoids. Endocrinology 118:1678-1681.
57. Strijbos, P. J., Hardwick, A. J., Relton, J. K., Carey, F., and Rothwell, N. J. (1992). Inhibition of central actions of cytokines on fever and thermogenesis by lipocortin-1 involves CRF. Am. J. Physiol. 263:E632-E636
58. Adashi, E. Y., Tucker, E. M., and Hsueh, A. J. W. (1984). Direct regulation of rat testicular steroidogenesis by neurohypophysial hormone. J. Biol. Chem. 259:5440-5446.
59. Wachsman, J. T. (1996). The beneficial effects of dietary restriction: Reduced oxidative damage and enhanced apoptosis. Mutation Res. 350:25-34.
60. Mehls, O., Tönshoff, B., Kovàcs, G., Mayer, C., Schurek, J., and Oh, J. (1993). Interaction between glucocorticoids and growth hormone. Acta. Paediatr. 82:77-82.
61. Suh, D. Y., Hunt, T. K., and Spencer, E. M. (1992). Insulin-like growth factor-I reverses the impairment of wound healing induced by corticosteroids in rats. Endocrinology 131:2399-2403.
62. Wehrenberg, W. B., Janowski, B. A., Piering, A. W., Culler, F., and Jones, K. L. (1990). Glucocorticoids: potent inhibitors and stimulators of growth hormone secretion. Endocrinology 126:3200-3203.
63. Planas, B., Kolb, P. E., Raskind, M. A., and Miller, M. A. (1995). Galanin-binding sites in the female rat brain are regulated across puberty yet similar to the male pattern in adulthood. Neuroendocrinol. 61:646-654.
64. Luo, J. and Murphy, L. J. (1989). Dexamethasone inhibits growth hormone induction of insulin-like growth factor-1 (IGF-1) messenger ribonucleic acid (mRNA) in hypophysectomized rats and reduces IGF-1 mRNA abundance in the intact rat. Endocrinology 125:165-171.
65. Kim, S. B., Yang, W. S., Lee, O. S., Lee, K. P., Park, J .S., and Na, D. S. (1996). Lipocortin-1 inhibits proliferation of cultured human mesangial cells. Nephron 74:39-44.
66. Wollenberg, G. K., LaMarre, J., Semple, E., Farber, E., Gauldie, J., and Hayes, M. A. (1991). Counteracting effects of dexamethasone and a₂-macroglobulin on inhibition of proliferation of normal and neoplastic rat hepatocytes by transforming growth factors-b type 1 and type 2. Intnl. J. Cancer 47:311-316.
67. Cooke, B. A., Platts, E. A., Abayasekera, R., Kurlak, L. O., Schulster, D., and Sullivan, M. H. F. (1989). Control of multiple transducing systems by LH which results in the modulation of adenylate cyclase, protein kinase C, lipoxygenases and cyclooxygenases. J. Reprod. Fert., Suppl. 37:139-145.
68. Cooke, B. A., Dirami, G., Chaudry, L., Choi, M. K. S., Abayasekera, D. R. E., and Phipp, L. (1991). Release of arachidonic acid and the effects of corticosteroids on steroidogenesis in rat testes Leydig cells. J. Steroid Biochem. Molec. Biol. 40:465-471.
69. Czerwinski, S. M., Kurowski, T. T., McKee, E. E., Zak, R., and Hickson, R. C. (1991). Myosin heavy chain turnover during cardiac mass changes by glucocorticoids. J. Appl. Physiol. 70:300-305.
70. Haddad, F., Bodell, P. W., McCue, S. A., Herrick, R. E., and Baldwin, K. M. (1993). Food restriction-induced transformations in cardiac functional and biochemical properties in rats. J. Appl. Physiol. 74:606-612.
71. Canman, C. E., Chen, C. Y., Lee, M. H., and Kastan, M. B. (1994). DNA damage responses: p53 induction, cell cycle perturbations, and apoptosis. Cold Spring Harbor Symp. Quant. Biol. 59:277-286.
72. Schwartzman, R. A. and Cidlowski, J. A. (1994). Glucocorticoid-induced apoptosis of lymphoid cells. Intnl. Arch. Allergy Immunol. 105:347-354.
73. Benedetti, A., Di Sario, A., Svegliati Baroni, G., and Jezequel, A. M. (1995). Transforming growth factor a1 increases the number of apoptotic bodies and decreases intracellular pH in isolated periportal and perivenular rat hepatocytes. Hepatol. 22:1488-1498.
74. Gantner, F., Leist, M., Jilg, S., Germann, P. G., Freudenberg, M. A., and Tiegs, G. (1995). Tumor necrosis factor-induced hepatic DNA fragmentation as an early marker of T cell-dependent liver injury in mice. Gastroenterol. 109:166-176.
75. Lee, J. M. and Bernstein, A. (1995). Apoptosis, cancer and the p53 tumor suppressor gene. Cancer Metastasis Rev. 14:149-161.
76. Witty, J. P., Lempka, T., Coffey, R. J., Jr., and Matrisian, L. M. (1995). Decreased tumor formation in 7,12-dimethylbenzanthracene-treated stromelysin-1 transgenic mice is associated with alterations in mammary epithelial cell apoptosis. Cancer Res. 55:1401-1406.
77. Mckanna, J. A. (1995). Lipocortin 1 in apoptosis: mammary regression. Anatom. Rec, 242:1-10.
78. Columbano, A. (1995). Cell death: Current difficulties in discriminating apoptosis from necrosis in the context of pathological processes in vivo. J. Cell. Biochem. 58:181-190.
79. O'Banion, M. K., Levenson, R. M., Brinckmann, U. G., and Young, D. A. (1992). Glucocorticoid modulation of transformed cell proliferation is oncogene specific and correlates with effects on c-myc levels. Mol. Endocrinol. 6:1371-1380.
80. Alexander, D. B., Goya, L., Webster, M. K., Haraguchi, T., and Firestone, G. L. (1993). Glucocorticoids coordinately disrupt a transforming growth factor a autocrine loop and suppress the growth of 13762NF-derived Con8 rat mammary adenocarcinoma cells. Cancer Res. 53:1808-1815.
81. Flower, R. L. (1988). Lipocortin and the mechanism of action of the glucocorticoids. Br. J. Pharmacol., 94:987-1015.
82. Selye, H. (1946). The general adaptation syndrome and the diseases of adaptation. J. Clin. Endocrinol. Metab. 6:117
83. Munck, A., Guyre, P. M., and Holbrook, N. J. (1984). Physiological functions of glucocorticoids in stress and their relation to pharmacological actions. Endocr. Rev, 5:25-44.
84. Flower, R. J. and Rothwell, N. J. (1994). Lipocortin-1: Cellular mechanisms and clinical relevance. Trends Pharmacol. Sci. 15:71-76.
85. Cover, P. O., Baanah-Jones, F., John, C. D., and Buckingham, J. C. (2002). Annexin 1 (lipocortin 1) mimics inhibitory effects of glucocorticoids on testosterone secretion and enhances effects of interleukin-1b. Endocrine Journal. 18:33-39.
86. Ritchie, R. H., Sun, X., and Dusting, G. J. (1999). Lipocortin-1 preserves myocardial responsiveness to beta-adrenergic stimulation in rat papillary muscle. Clin. Exp. Pharmacol. Physiol. 26:522-524.
87. Taylor, A. D., Philip, J. G., John, C. D., Cover, P. O., Morris, J. F., Flower, R. J., and Buckingham, J. C. (2000). Annexin 1 (lipocortin 1) mediates the glucocorticoid inhibition of cyclic adenosine 3',5'-monophosphate-stimulated prolactin secretion. Endocrinology 141:2209-2219.
88. Croxtall, J. D., Choudhury, Q., Tokumoto, H., and Flower, R. J. (1995). Lipocortin-1 and the control of arachidonic acid release in cell signaling. Glucocorticoids inhibit G protein-dependent activation of cPLA₂ activity. Biochem. Pharmacol. 50:465-474.
89. Croxtall, J. D., Choudhury, Q., Newman, S., and Flower, R. J. (1996). Lipocortin 1 and the control of cPLA₂ activity in A549 cells. Glucocorticoids block EGF stimulation of cPLA₂ phosphorylation. Biochem. Pharmacol. 52:351-356.
90. Loxley, H. D., Cowell, A. M., Flower, R. J., and Buckingham, J. C. (1993). Modulation of the hypothalamo-pituitary-adrenocortical responses to cytokines in the rat by lipocortin 1 and glucocorticoids: a role for lipocortin 1 in the feedback inhibition of CRF-41 release? Neuroendocrinol. 57:801-814.
91. Wang, W. and Creutz, C. E. (1994). Role of the amino-terminal domain in regulating interactions of annexin I with membranes: effects of amino-terminal truncation and mutagenesis of the phosphorylation sites. Biochem. 33:275-282.
92. Masferrer, J. L., Steibert, K., Zweifel, B., and Needleman, P. (1992). Endogenous glucocorticoids regulate an inducible cyclooxygenase enzyme. Proc. Natl. Acad. Sci. USA 89:3917-3921.
93. Masferrer, J. L., Zweifel, B. S., Manning, P. T., Hauser, S. D., Leahy, K. M., Smith, W. G., Isakson, P. C., and Seibert, K. (1994). Selective inhibition of inducible cyclooxygenase 2 in vivo is anti-inflammatory and nonulcerogenic. Proc. Natl. Acad. Sci. USA 91:3228-3232.
94. Seibert, K. and Masferrer, J. L. (1994). Role of inducible cyclooxygenase (COX-2) in inflammation. Receptor 4:17-23.
95. Salvemini, D., Manning, P. T., Zweifel, B. S., Seibert, K., Connor, J., Currie, M. G., Needleman, P., and Masferrer, J. L. (1995). Dual inhibition of nitric oxide and prostaglandin production contributes to the anti-inflammatory properties of nitric oxide synthase inhibitors. J. Clin. Invest. 96:301-308.
96. Schmidt, H. H. H. W., Lohmann, S. M., and Walter, U. (1993). The nitric oxide and cGMP signal transduction system: Regulation and mechanism of action. Biochim. Biophys. Acta 1178:153-175.
97. Geller, D. A., de Vera, M. E., Russell, D. A., Shapiro, R. A., Nussler, A. K., Simmons, R. L., and Billiar, T. R. (1995). A central role for IL-1ß in the in vitro and in vivo regulation of hepatic inducible nitric oxide synthase. IL-1ß induces hepatic nitric oxide synthesis. J. Immunol. 155:4890-4898.
98. Lilja, I., Dimberg, J., Sjodahl, R., Tagesson, C., and Gustafson-Svard, C. (1994). Effects of endotoxin and dexamethasone on group I and II phospholipase A₂ in rat ileum and stomach. Gut 35:40-45.
99. Wu, C. C., Croxtall, J. D., Perretti, M., Bryant, C. E., Thiemermann, C., Flower, R. J., and Vane, J. R. (1995). Lipocortin 1 mediates the inhibition by dexamethasone of the induction by endotoxin of nitric oxide synthase in the rat. Proc. Natl. Acad. Sci. USA 92:3473-3477.
100. Newman, S. P., Flower, R. J., and Croxtall, J. D. (1994). Dexamethasone suppression of IL-1ß-induced cyclooxygenase 2 expression is not mediated by lipocortin-1 in A549 cells. Biochem. Biophys. Res. Commun. 202:931-939.
101. Ikeda, M., Ezaki, M., Kokegouchi, S., and Ohmori, S. (1981). Studies on NADPH-dependent chloral hydrate reducing enzymes in rat liver cytosol. Biochem. Pharmacol. 30:1931-1939.
102. Ando, Y., Imamura, S., Owada, M. K., and Kannagi, R. (1991). Calcium-induced intracellular cross-linking of lipocortin I by tissue transaminase in A431 cells. J. Biol. Chem. 266:1101-1108.
103. Sakamoto, T., Repasky, W., Uchida, K., Hirata, A., and Hirata, F. (1996). Modulation of Cell Death Pathways to Apoptosis and Necrosis of H₂O₂-Treated Rat Thymocytes by Lipocortin-1. Biochem. Biophys. Res. Commun. 220:643-647.
104. Cato, A. C. and Wade, E. (1996). Molecular mechanisms of anti-inflammatory action of glucocorticoids. Bioessays 18:371-378.
105. Almawi, W. Y. and Melemedjian, O. K. (2002). Molecular mechanisms of glucocorticoid antiproliferative effects: antagonism of transcription factor activity by glucocorticoid receptor. Journal of Leukocyte Biology. 71:9-15.
106. Adcock, I. M. and Caramori, G. (2001). Cross-talk between pro-inflammatory transcription factors and glucocorticoids. Immunology & Cell Biology 79:376-384.
107. Haefner, B. (2002). NF-kB: arresting a major culprit in cancer. Drug Discovery Today 7:653-663.
108. Bours, V., Bentires-Alj, M., Hellin, A. C., Viatour, P., Robe, P., Delhalle, S., Benoit, V., and Merville, M. P. (2000). Nuclear factor-kB, cancer, and apoptosis. Biochem. Pharmacol. 60:1085-1089.
109. Shaulian, E. and Karin, M. (1920). AP-1 in cell proliferation and survival. Oncogene 20:2390-2400.
110. Perkins, N. D. (2000). The Rel/NF-kB family: friend and foe. Trends in Biochemical Sciences 25:434-440.
111. Tao, Y., Williams-Skipp, C., and Scheinman, R. I. (2001). Mapping of glucocorticoid receptor DNA binding domain surfaces contributing to transrepression of NF-kB and induction of apoptosis. Journal of Biological Chemistry 276:2329-2332.
112. Sakurai, H., Shigemori, N., Hisada, Y., Ishizuka, T., Kawashima, K., and Sugita, T. (1997). Suppression of NF-kB and AP-1 activation by glucocorticoids in experimental glomerulonephritis in rats: molecular mechanisms of anti-nephritic action. Biochimica et Biophysica Acta. 1362:252-262.
113. Bertrand, F., Atfi, A., Cadoret, A., L'Allemain, G., Robin, H., Lascols, O., Capeau, J., and Cherqui, G. (1998). A role for nuclear factor kB in the antiapoptotic function of insulin. Journal of Biological Chemistry 273:2931-2938.
114. Riccardi, C., Bruscoli, S., and Migliorati, G. (2002). Molecular mechanisms of immunomodulatory activity of glucocorticoids. Pharmacological Research 45:361-368.
115. Mittelstadt, P. R. and Ashwell, J. D. (2001). Inhibition of AP-1 by the glucocorticoid-inducible protein GILZ. Journal of Biological Chemistry 276:29603-29610.
116. Heufelder, A. E., Wenzel, B. E., and Bahn, R. S. (1993). Glucocorticoids modulate the synthesis and expression of a 72 kDa heat shock protein in cultured Graves' retroocular fibroblasts. Acta Endocrinol. 128:41-50.
117. Grombacher, T., Mitra, S., and Kaina, B. (1996). Induction of the alkyltransferase (MGMT) gene by DNA damaging agents and the glucocorticoid dexamethasone and comparison with the response of base excision repair genes. Carcinogenesis 17:2329-2336.
118. Bauer, J., Tran-Thi, T. A., Northoff, H., Hirsch, F., Schlayer, H. J., Gerok, W., and Heinrich, P. C. (1986). The acute-phase induction of a₂-macroglobulin in rat hepatocyte primary cultures: action of a hepatocyte-stimulating factor, triiodothyronine and dexamethasone. Eur. J. Cell Biol. 40:86-93.
119. Kurokawa, S., Ishibashi, H., Shirahama, M., Hayashida, K., Tsuchiya, Y., Sakaki, Y., and Niho, Y. (1988). Production of hepatocyte stimulating factor of rat Kupffer cells induced by lipopolysaccharide: partial characterization and effects on a₂ macroglobulin gene expression in cultured adult rat hepatocytes. J. Clin. Lab. Immunol. 25:131-137.
120. Marinkovic, S., Jahreis, G. P., Wong, G. G., and Baumann, H. (1989). IL-6 modulates the synthesis of a specific set of acute phase plasma proteins in vivo. J. Immunol. 142:808-812.
121. Dougall, W. C. and Nick, H. S. (1991). Manganese superoxide dismutase: a hepatic acute phase protein regulated by interleukin-6 and glucocorticoids. Endocrinology 129:2376-2384.
122. Hocke, G. M., Barry, D., and Fey, G. H. (1992). Synergistic action of interleukin-6 and glucocorticoids is mediated by the interleukin-6 response element of the rat a₂ macroglobulin gene. Mol. Cell. Biol. 12:2282-2294.
123. Garcia-Leme, J., Fortes, Z. B., Sannomiya, P., and Farsky, S. P. (1992). Insulin, glucocorticoids and the control of inflammatory responses. Agents Actions 36:99-118.
124. Zacharchuk, C. M., Mercerp, M., Chakaborti, P. K., Simons, S. S., Jr., and Ashwell, J. D. (1990). Programmed T lymphocyte death. Cell-activated and steroid-induced pathways are mutually antagonistic. J. Immunol. 145:4037-4045.
125. King, L. B. and Ashwell, J. D. (1994). Thymocyte and T cell apoptosis: is all death created equal? Thymus 23:209-230.
126. Croxtall, J. D. and Flower, R. J. (1992). Lipocortin 1 mediates dexamethasone-induced growth arrest of the A549 lung adenocarcinoma cell line. Proc. Natl. Acad. Sci. USA 89:3571-3575.
127. Wattenberg, L. W. and Estensen, R. D. (1996). Chemopreventive effects of myo-inositol and dexamethasone on benzo[a]pyrene and 4-(methylnitrosoamino)-1-(3-pyridyl)-1- butanone-induced pulmonary carcinogenesis in female A/J mice. Cancer Res. 56:5132-5135.
128. Hofmann, J., Kaiser, U., Maasberg, M., and Havemann, K. (1995). Glucocorticoid receptors and growth inhibitory effects of dexamethasone in human lung cancer cell lines. Eur. J. Cancer 31A: 2053-2058.
129. Duncan, G. S., Peers, S. H., Carey, F., Forder, R., and Flower, R. J. (1993). Dexamethasone inhibits induction of liver tumor necrosis factor-a mRNA and liver growth induced by lead nitrate and ethylene dibromide. Am. J. Pathol. 145:951-958.
130. Rao, M. S. and Subbarao, V. (1997). Effect of dexamethasone on ciprofibrate-induced cell proliferation and peroxisome proliferation. Fundam. Appl. Toxicol. 35:78-83.
131. Roseng, L. E. and Rivedal, E. (1993). Effect of glucocorticoids on TPA-induced inhibition of gap-junctional communication and morphological transformation in Syrian Hamster embryo cells. Cancer Lett. 72:25-30.
132. Kwiatkowski, A. P., Baker, T. K., and Klaunig, J. E. (1994). Comparison of glucocorticoid-mediated changes in the expression and function of rat hepatocyte gap junctional proteins. Carcinogenesis 15:1753-1757.
133. Ren, P., de Feijter, A. W., Paul, D. L., and Ruch, R. J. (1994). Enhancement of liver cell gap junction protein expression by glucocorticoids. Carcinogenesis 15:1807-1813.
134. Slaga, T. J., DiGiovanni, J., Winberg, L. D., and Budunova, I. V. (1995). Skin carcinogenesis: characteristics, mechanisms, and prevention. Prog. Clin. Biol. Res. 391:1-20.
135. Gaynon, P. S. and Lustig, R. H. (1995). The use of glucocorticoids in acute lymphoblastic leukemia of childhood. Molecular, cellular, and clinical considerations. J. Pediat. Hematol. Oncol. 17:1-12.
136. McEwen, B. S. and Sapolsky, R. M. (1995). Stress and cognitive function. Curr. Opinion Neurobiol. 5:205-216.
137. Rothwell, N. J. and Relton, J. K. (1993). Involvement of cytokines in acute neurodegeneration in the CNS. Neurosci. Biobehav. Rev. 17:217-227.
138. Sapolsky, R., Krey, L., and McEwen, B. (1993). The neuroendocrinology of stress and aging: The glucocorticoid cascade hypothesis. Endocr. Rev. 7:284-302.
139. Stein-Behrens, B A. and Sapolsky, R. M. (1992). Stress, glucocorticoids and aging. Aging Clin. Exp. Res. 4:197-210.
140. Landfield, P. W. and Eldridge, J. C. (1994). Evolving aspects of the glucocorticoid hypothesis of brain aging: hormonal modulation of neuronal calcium homeostasis. Neurobiol. Aging 15:579-588.
141. Starkman, M. N., Schteingart, D. E., and Schork, M. A. (1986). Cushing's syndrome after treatment: changes in cortisol and ACTH levels, and amelioration of the depressive syndrome. Psychiat. Res. 19:177-188.
142. Newcomer, J. W., Craft, S., Hershey, T., Askins, K., and Bardgett, M. E. (1994). Glucocorticoid-induced impairment in declarative memory performance in adult humans. J. Neurosci. 14:2047-2053.
143. Breitner, J. C. S., Gau, B. A., Welsh, K. A., Plassman, B. L., McDonald, W. M., Helms, M. J., and Amthony, J. C. (1994). Inverse association of anti-inflammatory treatments and Alzheimer's disease: Initial results of a co-twin control study. Neurol. 44:227-232.
144. Stevens, T. R., Smith, S. F., and Rampton, D. S. (1993). Antibodies to human recombinant lipocortin-I in inflammatory bowel disease. Clin. Sci. 84:381-386.
145. Rothwell, N. J. and Relton, J. K. (1993). Involvement of interleukin-1 and lipocortin-1 in ischaemic brain damage. Cerebrovascular Brain Metab. Rev. 5:178-198.
146. Welsh, T. H. J., Bambino, T. H., and Hsueh, A. J. W. (1982). Mechanism of glucocorticoid-induced suppression of testicular androgen biosynthesis in vitro. Biol. Reprod. 27:1138-1146.
147. Bambino, T. H. and Hsueh, A. J. W. (1981). Direct Inhibitory effect of glucocorticoids upon testicular luteinizing hormone receptor and steroidogenesis in vivo and in vitro. Endocrinology 108:2142-2147.
148. Gao, H. B., Shan, L. X., Monder, C., and Hardy, M. P. (1996). Suppression of endogenous corticosterone levels in vivo increases the steroidogenic capacity of purified rat Leydig cells in vitro. Endocrinology 137:1714-1718.
149. Hsueh, A. J. W. and Erickson, G. F. (1978). Glucocorticoid inhibition of FSH-induced estrogen production in cultured rat granulosa cells. Steroids 32:639-648.
150. Inazu, N., Iwata, N., and Satoh, T. (1990). Inhibitory effect of glucocorticoid and stimulatory effect of human chorionic gonadotropin on ovarian carbonyl reductase in rats. Life Sci. 46:841-848.
151. Baldwin, D. M. and Sawyer, C. H. (1974). Effects of dexamethasone on LH release and ovulation in the cyclic rat. Endocrinology 94:1397-1403.
152. Kamel, F. and Kubajak, C. L. (1987). Modulation of gonadotropin secretion by corticosterone: interaction with gonadal steroids and mechanism of action. Endocrinology 121:561-568.
153. Lopez-Calderon, A., Ariznavarreta, C., Calderon, M. D., Tresguerres, J. A., and Gonzalez-Quijano, M. I. (1989). Role of the adrenal cortex in chronic stress-induced inhibition of prolactin secretion in male rats. J. Endocrinol. 120:269-273.
154. Lopez-Calderon, A., Ariznavarreta, C., Calderon, M. D., and Tresguerres, J. A. (1987). Gonadotropin inhibition during chronic stress: role of the adrenal gland. J. Steroid Biochem. 27:609-614.
155. Rivier, C. and Vale, W. (1984). Influence of corticotropin-releasing factor on reproductive functions in the rat. Endocrinology 114:914-921.
156. Rivier, C. and Vale, W. (1985). Effect of long-term administration of corticotropin-releasing factor on the pituitary-adrenal and pituitary gonadal axis in the male rat. J. Clin. Invest. 75:689-694.
157. Kalant, N., Stewart, J., and Kaplan, R. (1988). Effect of diet restriction on glucose metabolism and insulin responsiveness in aging rats. Mech. Ageing Devel. 46:89-104.
158. Bodkin, N. L., Ortmeyer, H. K., and Hansen, B. C. (1995). Long-term dietary restriction in older-aged rhesus monkeys: effects on insulin resistance. J. Gerontol. 50:B142-B147
159. Ohneda, M., Inman, L. R., and Unger, R. H. (1995). Caloric restriction in obese pre-diabetic rats prevents beta-cell depletion, loss of beta-cell GLUT 2 and glucose incompetence. Diabetologia 38:173-179.
160. Lewis, S. E., Goldspink, D. F., Phillips, J. G., Merry, B. J., and Holehan, A. M. (1985). The effects of aging and chronic dietary restriction on whole body growth and protein turnover in the rat. Exp. Gerontol. 20:253-263.
161. Wolf, N. S., Penn, P. E., Jiang, D., Fei, R. G., and Pendergrass, W. R. (1995). Caloric restriction: conservation of in vivo cellular replicative capacity accompanies life span extension in mice. Exp. Cell Res. 217:317-323.
162. Forster, M. J., Dubey, A., Dawson, K. M., Stutts, W. A., Lal, H., and Sohal, R. S. (1996). Age-related losses of cognitive function and motor skills in mice are associated with oxidative protein damage in the brain. Proc. Natl. Acad. Sci. USA 93:4765-4769.
163. Lal, H., Forster, M. J., and Sohal, R. S. (1995). Oxidative brain damage in aged mice. Protection by caloric reduction. Annal. NY. Acad. Sci. 765:308
164. Holehan, A. M. and Merry, B. J. (1985). Modification of the oestrous cycle hormonal profile by dietary restriction. Mech. Ageing Devel. 32:63-76.
165. Keenan, K. P., Soper, K. A., Hertzog, P. R., Gumprecht, L. A., Smith, P. F., Mattson, B. A., Ballam, G. C., and Clark, R. L. (1995). Diet, overfeeding, and moderate dietary restriction in control Sprague-Dawley rats: II. Effects on age-related proliferative and degenerative lesions. Toxicologic Pathol. 23: 287-302.
166. Reul, J. M., Van den Bosch, F. R., and De Kloet, E. R. (1987). Differential response of type I and type II corticosteroid receptors to changes in plasma steroid level and circadian rhythmicity. Neuroendocrinol. 45:407-412.
167. Ma, Q., Dannan, G. A., Guengerich, F. P., and Yang, C. S. (1989). Similarities and differences in the regulation of hepatic cytochrome P-450 enzymes by diabetes and fasting in male rats. Biochem. Pharmacol. 38:3179-3184.
168. Masoro, E. J., Shimokawa, I., and Yu, B. P. (1991). Retardation of the aging processes in rats by food restriction. Annal. NY. Acad. Sci. 621:337-352.
169. Sell, D. R., Lane, M. A., Johnson, W. A., Masoro, E. J., Mock, O. B., Reiser, K. M., Fogarty, J. F., Cutler, R. G., Ingram, D. K., Roth, G. S., and Monnier, V. M. (1996). Longevity and the genetic determination of collagen glycoxidation kinetics in mammalian senescence. Proc. Natl. Acad. Sci. USA 93:485-490.
170. Sohal, R. S., Agarwal, S., Candas, M., Forster, M. J., and Lal, H. (1994). Effect of age and caloric restriction on DNA oxidative damage in different tissues of C57BL/6 mice. Mech. Ageing Devel. 76:215-224.
171. Djuric, Z., Lu, M. H., Lewis, S. M., Luongo, D. A., Chen, X. W., Heilbrun, L. K., Reading, B. A., Duffy, P. H., and Hart, R. W. (1992). Oxidative damage levels in rats fed low-fat, high-fat, or calorie-restricted diets. Toxicol. Appl. Pharmacol. 115:156-160.
172. NTP (1996). NTP Technical Report Series No. 446. Toxicology and Carcinogenesis Studies of 1-trans-delta9-Tetrahydrocannabinol (CAS No. 1972-08-3) in F344/N Rats and B6C3F1 Mice. National Toxicology Program, USDHHS, PHS, NIH, Research Triangle Park, NC.
173. Cadenas, S., Rojas, C., Perez-Campo, R., Lopez-Torres, M., and Barja, G. (1994). Caloric and carbohydrate restriction in the kidney: effects on free radical metabolism. Exp. Gerontol. 29:77-88.
174. Aidoo, A., Desai, V. G., Lyn-Cook, L. E., Chen, J. J., Feuers, R. J., and Casciano, D. A. (1999). Attenuation of bleomycin-induced Hprt mutant frequency in female and male rats by calorie restriction. Mutation Research 430:155-163.
175. Desai, V. G., Aidoo, A., Li, J., Lyn-Cook, L. E., Casciano, D. A., and Feuers, R. J. (2000). Effects of bleomycin on liver antioxidant enzymes and the electron transport system from ad libitum-fed and dietary-restricted female and male Fischer 344 rats. Nutrition & Cancer 36:42-51.
176. Gredilla, R., Barja, G., and Lopez-Torres, M. (2001). Effect of short-term caloric restriction on H₂O₂ production and oxidative DNA damage in rat liver mitochondria and location of the free radical source. Journal of Bioenergetics & Biomembranes 33:279-287.
177. Duffy, P. H., Feuers, R. J., Leakey, J. E. A., Nakamura, K. D., Turturro, A., and Hart, R. W. (1989). Effect of chronic caloric restriction on the physiological variables related to energy metabolism in the Fischer 344 rat. Mech. Ageing Devel. 48:117-133.
178. Pendergrass, W. R., Li, Y., Jiang, D., Fei, R. G., and Wolf, N. S. (1995). Caloric restriction: conservation of cellular replicative capacity in vitro accompanies life span extension in mice. Exp. Cell Res. 217:309-316.
179. Sonntag, W. E., Xu, X., Ingram, R. L., and D'Costa, A. (1995). Moderate caloric restriction alters the subcellular distribution of somatostatin mRNA and increases growth hormone pulse amplitude in aged animals. Neuroendocrinol. 61:601-608.
180. Hynes, M. A., Van Wyk, J. J., Brooks, P. J., D'Ercole, A. J., Jansen, M., and Lund, P. K. (1987). Growth hormone dependence of somatomedin-C/insulin-like growth factor-I and insulin-like growth factor-II messenger ribonucleic acids. Mol. Endocrinol. 1:233-242.
181. Westin, S., Tollet, P., Strom, A., Mode, A., and Gustafsson, J. A. (1992). The role and mechanism of growth hormone in the regulation of sexually dimorphic-P450 enzymes in rat liver. J. Steroid Biochem. Molec. Biol. 43:1045-1053.
182. Breese, C. R., Ingram, R. L., and Sonntag, W. (1991). Influence of age and long-term dietary restriction on plasma insulin-like growth factor-1 (IGF-1), IGF-1 gene expression, and IGF-1 binding proteins. J. Gerontol. 46:B180-B187
183. Manjgaladze, M., Chen, S., Frame, L. T., Seng, J .E., Duffy, P. H., Feuers, R. J., Hart, R. W., and Leakey, J. E. A. (1993). Effects of caloric restriction on rodent drug and carcinogen metabolizing enzymes: Implications for mutagenesis and cancer. Mutation Res. 295:201-222.
184. Prasanna, H. R., Lu, M. H., and Hart, R. W. (1990). Status of dehydroepiandrosterone and hepatic metabolism of aflatoxin B₁ in food restricted rats. Biochem. Arch. 6:419-427.
185. Bronson, F. H. (1986). Food-restricted, prepubertal, female rats: rapid recovery of luteinizing hormone pulsing with excess food, and full recovery of pubertal development with gonadotropin-releasing hormone. Endocrinology 118:2483-2487.
186. Holehan, A. M. and Merry, B. J. (1985). The control of puberty in the dietary restricted female rat. Mech. Ageing Devel. 32:179-191.
187. Bronson, F. H. and Marsteller, F. A. (1985). Effect of short-term food deprivation on reproduction in female mice. Biol. Reprod. 33:660-667.
188. Holehan, A. M. and Merry, B. J. (1985). Lifetime breeding studies in fully fed and dietary restricted female CFY Sprague-Dawley rats. 1. Effect of age, housing conditions and diet on fecundity. Mech. Ageing Devel. 33:19-28.
189. Chapin, R. E., Gulati, D. K., Fail, P. A., Hope, E., Russell, S. R., Heindel, J. J., George, J. D., Grizzle, T. B., and Teague, J. L. (1993). The effects of feed restriction on reproductive function in Swiss CD-1 mice. Fundam. Appl. Toxicol. 20:15-22.
190. Woodside, B. (1991). Effects of food restriction on the length of lactational diestrus in rats. Horm. Behav. 25:70-83.
191. Young, C. M. and Rasmussen, K. M. (1985). Effects of varying degrees of chronic dietary restriction in rat dams on reproductive and lactational performance and body composition in dams and their pups. Am. J. Clin. Nutr. 41:979-987.
192. Sisk, C. L. and Bronson, F. H. (1986). Effects of food restriction and restoration on gonadotropin and growth hormone secretion in immature male rats. Biol. Reprod. 35:554-561.
193. Seng, J. E., Gandy, J., Turturro, A., Lipman, R., Bronson, R. T., Parkinson, A., Johnson, W., Hart, R. W., and Leakey, J. E. A. (1996). Effects of caloric restriction on expression of testicular cytochrome P450 enzymes associated with the metabolic activation of carcinogens. Arch. Biochem. Biophys. 335:42-52.
194. Johnson, L., May, M. R., Busbee, D. L., and Williams, J. D. (1992). Effect of age and dietary restriction on daily sperm production and number and transit time of epididimal spermatozoa in the mouse. Age 15:65-72.
195. Chapin, R. E., Gulati, D. K., Barnes, L. H., and Teague, J. L. (1993). The effects of feed restriction on reproductive function in Sprague-Dawley rats. Fundam. Appl. Toxicol. 20:23-29.
196. Thurman, J. D., Bucci, T., Hart, R. W., and Turturro, A. (1994). Survival, body weight and spontaneous neoplasms in ad libitum fed and dietary restricted Fischer 344 rats. Toxicologic Pathol. 22:1-9.
197. Bronson, F. H. (1982). Relative effects of exercise, diet, and female stimulation on sexual aging of male mice. J. Gerontol. 37: 555-559.
198. Engelman, R. W., Day, N. K., and Good, R. A. (1993). Calories, cell proliferation, and proviral expression in autoimmunity and cancer. Proc. Soc. Exp. Biol. Med. 203:13-17.
199. Pashko, L. L. and Schwartz, A. G. (1992). Reversal of food restriction-induced inhibition of mouse skin tumor promotion by adrenalectomy. Carcinogenesis 13:1925-1928.
200. Schwartz, A. G. and Pashko, L. L. (1994). Role of adrenocortical steroids in mediating cancer-preventive and age-retarding effects of food restriction in laboratory rodents. J. Gerontol. 49:B37-B41
201. Himeno, Y., Engelman, R. W., and Good, R. A. (1992). Influence of calorie restriction on oncogene expression and DNA synthesis during liver regeneration. Proc. Natl. Acad. Sci. USA 89:5497-5501.
202. Grasl-Kraupp, B., Bursch, W., Ruttkay-Nedecky, B., Wagner, A., Lauer, B., and Schulte-Hermann, R. (1994). Food restriction eliminates preneoplastic cells through apoptosis and antagonizes carcinogenesis in rat liver. Proc. Natl. Acad. Sci. USA 91:9995-9999.
203. Muskhelishvili, L., Hart, R. W., Turturro, A., and James, S. J. (1995). Age-related changes in the intrinsic rate of apoptosis in livers of diet-restricted and ad libitum-fed B6C3F1 mice. Am. J. Pathol. 147:20-24.
204. Kari, F., Hatch, G., Slade, R., Crissman, K., Simeonova, P. P., and Luster, M. (1997). Dietary restriction mitigates ozone-induced lung inflammation in rats: a role for endogenous antioxidants. Am. J. Respir. Cell Mol. Biol. 17:740-747.
205. Dong, W., Selgrade, M. K., Gilmour, I. M., Lange, R. W., Park, P., Luster, M. I., and Kari, F. W. (1998). Altered alveolar macrophage function in calorie-restricted rats. Am. J. Respir. Cell Mol. Biol. 19:462-469.
206. O'Steen, W. K. and Landfield, P. W. (1991). Dietary restriction does not alter retinal aging in the Fischer 344 rat. Neurobiol. Aging 12:455-462.
207. Green, M. W., Rogers, P. J., Elliman, N. A., and Gatenby, S. J. (1994). Impairment of cognitive performance associated with dieting and high levels of dietary restraint. Physiol. Behav. 55:447-452.
208. Duffy, P. H., Feuers, R. J., Pipkin, J. L., Berg, T. F., Devine, B., Leakey, J. E. A., and Hart, R. W. (1995). The effect of aging on the physiological response of rodents to drug toxicity. In: Dietary Restriction. Implications for the Design and Interpretation of Toxicity and Carcinogenicity Studies, edited by D. A. Neumann, et al, pp. 127-140. ILSI, Washington, DC.
209. Keenan, K. P., Laroque, P., Ballam, G. C., Soper, K. A., Dixit, R., Mattson, B. A., Adams, S. P., and Coleman, J. B. (1996). The effects of diet, ad libitum overfeeding, and moderate dietary restriction on the rodent bioassay: The uncontrolled variable in safety assessment. Toxicologic Pathol. 24:757-768.
210. Leakey, J. E. A., Seng, J. E., Manjgaladze, M., Kozlovskaya, N., Xia, S., Lee, M. -Y., Frame, L. T., Chen, S., Rhodes, C. L., Duffy, P. H., and Hart, R. W. (1995). Influence of caloric intake on drug metabolizing enzyme expression: Relevance to tumorigenesis and toxicology testing. In: Dietary Restriction. Implications for the Design and Interpretation of Toxicity and Carcinogenicity Studies, edited by D. A. Neumann, et al, pp. 167-180. ILSI, Washington, DC.
211. Satta, A., Faedda, R., Olmeo, N. A., Soggia, G., Branca, G. F., and Bartoli, E. (1984). Studies on the nephron segment with reduced sodium reabsorption during starvation natriuresis. Renal Physiology 7:283-292.
212. Maoz, E., Shamiss, A., Peleg, E., Salzberg, M., and Rosenthal, T. (1992). The role of atrial natriuretic peptide in natriuresis of fasting. J. Hypertent. 10:1041-1044.
213. Verbaeys, A., Ringoir, S., Van Maele, G., and Lameire, N. (1995). Influence of feeding, blood sampling method and type of anaesthesia on renal function parameters in the normal laboratory rat. Urol. Res. 22:377-382.
214. Fullerton, M. J., Krozowski, Z. S., and Funder, J. W. (1991). Adrenalectomy and dexamethasone administration: effect on atrial natriuretic peptide synthesis and circulating forms. Mol. Cell. Endocrinol. 82:33-40.
215. Behrend, E. N. and Kemppainen, R. J. (1997). Glucocorticoid therapy. Pharmacology, indications, and complications. Vet. Clin. North America. Small Animal Pract. 27:187-213.
216. Mathis, J. M., Houser, W. H., Bresnick, E., Cidlowski, J. A., Hines, R. N., Prough, R. A., and Simpson, E. R. (1989). Glucocorticoid regulation of the rat cytochrome P450c (P450IA1) gene: receptor binding within Intron 1. Arch. Biochem. Biophys. 269:93-105.
217. Jaiswal, A. K., Haaparanta, T., Luc, P.-V., Schembri, J., and Adesnik, M. (1990). Glucocorticoid regulation of a phenobarbital-inducible cytochrome P-450 gene: the presence of a functional glucocorticoid response element in the 5'-flanking region of the CYP2B2 gene. Nucleic Acid Res. 18:4237-4242.
218. Prough, R. A., Linder, M. W., Pinaire, J. A., Xiao, G. H., and Falkner, K. C. (1996). Hormonal regulation of hepatic enzymes involved in foreign compound metabolism. FASEB J. 10:1369-1377.
219. Seng, J. E., Agrawal, N., Horsley, E. M. T., Leakey, T. I., Schere, E. M., Xia, S., Allaben, W. T., and Leakey, J. E. A. (2003). Toxicokinetics of chloral hydrate in ad libitum -fed, and dietary-controlled and calorically restricted male B6C3F₁ mice following short-term exposure. Toxicol. Appl. Pharmacol. 193:281-292.
220. Chou, M. W., Kong, J., Chung, K. -T., and Hart, R. W. (1993). Effect of caloric restriction on the metabolic activation of xenobiotics. Mutation Res. 295:223-235.
221. Shaddock, J. G., Feuers, R. J., Chou, M. W., Pegram, R. A., and Casciano, D. A. (1993). Effects of aging and caloric restriction on the genotoxicity of 4 carcinogens in the in vitro rat hepatocyte/DNA repair assay. Mutation Res. 295:19-30.
222. Haley-Zitlin, V. and Richardson, A. (1993). Effect of dietary restriction on DNA repair and DNA damage. Mutation Res. 295:237-245.
223. Allaben, W. T., Chou, M. W., and Pegram, R. A. (1991). Dietary restriction and toxicological endpoints: An historical overview. In: Biological Effects of Dietary Restriction, edited by L. Fishbein, pp. 27-41. Springer-Verlag, New York.
224. Chou, M. W., Shaddock, J. G., Kong, J., Hart, R. W., and Casciano, D. A. (1995). Effect of dietary restriction on partial hepatectomy-induced liver regeneration of aged F344 rats. Cancer Lett. 91:191-197.
225. Kari, F. W. and Abdo, K. B. (1995). The sensitivity of the NTP bioassay for carcinogen hazard evaluation can be modulated by dietary restriction. In: Dietary restriction. Implications for the design and interpretation of toxicity and carcinogenicity studies, edited by R. W. Hart, et al, pp. 63-78. ILSI Press, Washington, DC.
226. Casciano, D. A., Chou, M., Lyn-Cook, L. E., and Aidoo, A. (1996). Calorie restriction modulates chemically induced in vivo somatic mutation frequency. Environmental & Molecular Mutagenesis 27:162-164.
227. Fu, P. P., Dooley, K. L., VonTungeln, L. S., Bucci, T., Hart, R. W., and Kadlubar, F. F. (1994). Caloric restriction profoundly inhibits liver tumor formation after initiation by 6-nitrochrysene in male mice. Carcinogenesis 15:159-161.
228. Turturro, A., Duffy, P. H., and Hart, R. W. (1993). Modulation of toxicity by diet and dietary macronutrient restriction. Mutation Res. 295:151-164.
229. Seilkop, S. K. (1995). The effect of body weight on tumor incidence and carcinogenicity testing in B6C3F₁ mice and F344 rats. Fundam. Appl. Toxicol. 24:247-259.
230. Hart, R. W., Keenan, K., Turturro, A., Abdo, K. M., Leakey, J. E. A., and Lyn-Cook, B. (1995). Caloric restriction and toxicity. Fundam. Appl. Toxicol. 25:184-195.
231. Leakey, J. E. A., Seng, J. E., and Allaben, W. T. (2003). Body weight considerations in the B6C3F₁ mouse and the use of dietary control to standardize background tumor incidence in chronic bioassays. Toxicol. Appl. Pharmacol. 193:237-265.
232. Turturro, A., Duffy, P., Hart, R. W., and Allaben, W. T. (1996). Rational use of dietary control in toxicity studies - B6C3F₁ mouse. Toxicologic Pathol. 24:769-775.
233. Turturro, A., Blank, K., Murasko, D., and Hart, R. (1994). Mechanisms of caloric restriction affecting aging and disease. Annal. NY. Acad. Sci. 719:159-170.
234. Bronson, F. H. (1984). Energy allocation and reproductive development in wild and domestic house mice. Biol. Reprod. 31:83-88.
235. Bronson, F. H. (1988). Mammalian reproductive strategies: genes, photoperiod and latitude. Reprod. Nutr. Develop. 28:335-347.
236. Merry, R. J. and Holehan, A. M. (1991). The effect of dietary restriction on the endocrine control of reproduction. In: Biological Effects of Dietary Restriction, edited by L. Fishbein, pp. 140-146. Springer-Verlag, New York.
237. Graves, J. L. (1993). The costs of reproduction and dietary restriction: parallels between insects and mammals. Growth Develop. Aging 57:233-249.
238. Turturro, A., Duffy, P. H., and Hart, R. W. (1995). The effect of caloric modulation on toxicity studies. In: Dietary Restriction: Implications for the Design and Interpretation of Toxicity and Carcinogenicity Studies, edited by R. W. Hart, et al, pp. 1-2. ILSI Press, Washington, DC.
239. Haseman, J. K., Bourbina, J., and Eustis, S. L. (1994). Effect of individual housing and other experimental design factors on tumor incidence in B6C3F₁ mice. Fundam. Appl. Toxicol. 23:44-52.
240. Haseman, J. K. (1985). Issues in carcinogenicity testing: Dose selection. Fundam. Appl. Toxicol. 5:66-78.
241. Tokuyama, K. and Himms-Hagen, J. (1987). Increased sensitivity of the genetically obese mouse to corticosterone. Am. J. Physiol. 252202:E202-E208
242. Dubuc, P. U. (1992). Interactions between insulin and glucocorticoids in the maintenance of genetic obesity. Am. J. Physiol. 263: E550-E555
243. Lefkowith, J. B. and Klahr, S. (1996). Polyunsaturated fatty acids and renal disease. Proc. Soc. Exp. Biol. Med., 213:13-23.
244. Ishiyama, H., Ogino, K., and Hobara, T. (1995). Role of Kupffer cells in rat liver injury induced by diethyldithiocarbamate. Eur. J. Pharmacol. 292:135-141.
245. Armendariz-Borunda, J., Seyer, J. M., Postlethwaite, A. E., and Kang, A. H. (1991). Kupffer cells from carbon tetrachloride-injured rat livers produce chemotactic factors for fibroblasts and monocytes: the role of tumor necrosis factor-a. Hepatol. 14:895-900.
246. Edwards, M. J., Keller, B. J., Kauffman, F. C., and Thurman, R. G. (1993). The involvement of Kupffer cells in carbon tetrachloride toxicity. Toxicol. Appl. Pharmacol. 119:275-279.
247. Dunn, S. E., Kari, F. W., French, J., Leininger, J. R., Travlos, G., Wilson, R., and Barrett, J. C. (1997). Dietary restriction reduces insulin-like growth factor I levels, which modulates apoptosis, cell proliferation, and tumor progression in p53-deficient mice. Cancer Res. 57:4667-4672.
248. Berrigan, D., Perkins, S. N., Haines, D. C., and Hursting, S. D. (2002). Adult-onset calorie restriction and fasting delay spontaneous tumorigenesis in p53-deficient mice. Carcinogenesis 23:817-822.
249. Albanes, D. (1987). Total calories, body weight, and tumor incidence in mice. Cancer Res. 47:1987-1992.
250. Seng, J. E., Allaben, W. T., Nichols, M. L., Bryant, B. D., Ulmer, C., Contrera, J. F., and Leakey, J. E. A. (1998). Putting dietary control to the test: Increasing bioassay sensitivity by reducing variability. Lab Animal 27:35-38.
251. NTP (2002). NTP Technical Report Series No. 503. Toxicology and Carcinogenesis Studies of Chloral Hydrate (CAS No. 302-17-0) in Male (ad libitum and dietary controlled) B6C3F₁ Mice (Gavage study). National Toxicology Program, USDHHS, PHS, NIH, Research Triangle Park, NC.
252. Leakey, J. E. A., Seng, J. E., Latendresse, J. R., Hussain, N., Allen, L. J., and Allaben, W. T. (2003). Dietary controlled carcinogenicity study of chloral hydrate in Male B6C3F₁. Toxicol. Appl. Pharmacol.193:66-280.
253. Poole, T. M. and Drinkwater, N. R. (1996). Strain dependent effects of sex hormones on hepatocarcinogenesis in mice. Carcinogenesis 17:191-196.
254. Kemp, C. J. and Drinkwater, N. R. (1990). The androgen receptor and liver tumor development in mice. Prog. Clin. Biol. Res. 331:203-214.
255. Poole, T. M. and Drinkwater, N. R. (1995). Hormonal and genetic interactions in murine hepatocarcinogenesis. Prog. Clin. Biol. Res. 391:187-194.
256. Jeong, K. H., Jacobson, L., Widmaier, E. P., and Majzoub, J. A. (1999). Normal suppression of the reproductive axis following stress in corticotropin-releasing hormone-deficient mice. Endocrinology 140:1702-1708.
257. McClain, R. M. (1995). Phenobarbital mouse liver tumors: implications of hepatic tumor promotion for cancer risk assessment. Prog. Clin. Biol. Res. 391:325-336.
258. Melnick, R. L., Kohn, M. C., and Portier, C. J. (1996). Implications for risk assessment of suggested nongenotoxic mechanisms of chemical carcinogenesis. Environ. Hlth. Persp. 104 Suppl 1:123-134.
259. Ward, J. M., Shibata, M. A., and Devor, D. E. (1996). Emerging issues in mouse liver carcinogenesis. Toxicologic Pathology. 24:129-137.
260. Befeler, A. S. and Di Bisceglie, A. M. (2002). Hepatocellular carcinoma: diagnosis and treatment. Gastroenterology 122:1609-1619.
261. Simmonds, P. (2001). Reconstructing the origins of human hepatitis viruses. Philosophical Transactions of the Royal Society of London - Series B: Biological Sciences 356:1013-1026.
262. Holmes-McNary, M. (2001). Impact factors on development of cirrhosis and subsequent hepatocellular carcinoma. Compendium of Continuing Education in Dentistry 22:19-33.
263. Sheldon, W. G., Bucci, T. J., Hart, R. W., and Turturro, A. (1995). Age-related neoplasia in a lifetime study of ad libitum-fed and food restricted B6C3F₁ mice. Toxicologic Pathol. 23:458-476.
264. Hengstler, J. G., Van der Burg, B., Steinberg, P., and Oesch, F. (1999). Interspecies differences in cancer susceptibility and toxicity. Drug Metab. Rev. 31:917-970.
265. Maronpot, R. R., Haseman, J. K., Boorman, G. A., Eustis, S. E., Rao, G. N., and Huff, J. E. (1987). Liver lesions in B6C3F₁ mice: the National Toxicology Program, experience and position. Arch. Toxicol. Suppl. 10:10-26.
266. Hart, R. W., Leakey, J. E., Chou, M., Duffy, P. H., Allaben, W. T., and Feuers, R. J. (1992). Modulation of chemical toxicity by modification of caloric intake. Adv. Exp. Med. Biol. 322:73-81.

Glossary

Apoptosis: Apoptosis is a process of programmed cell death triggered by either external hormonal signals or internal damage, which is characterized by ordered degradation of chromatin and the rapid phagocytosis of cellular debris without the release of inflammatory mediators. Thus, apoptosis differs from necrotic cell death in that there is no associated inflammation or compensatory mitogenesis.

Body weight reduction: In general, body weight reductions resulting from dietary restriction are reductions in body weight gain relative to corresponding ad libitum -fed control animals. That is the restricted animals are gaining weight but at a slower rate. However, individual animals, particularly older rodents on long-term dietary restriction studies, may actually lose weight on a short-term basis, but generally not on a long-term basis unless the weight-loss is associated with morbidity.

Dietary restriction: The term is used loosely here to incorporate both food restriction and caloric restriction. Caloric restriction is defined as the balanced and moderate reduction of the carbohydrate, protein and fat content of a diet without a reduction in vitamin or micronutrient content. Caloric restriction by 10 -40% of ad libitum food consumption has typically been used in aging studies. Food restriction, where total food intake is reduced, is simpler to perform and has been used in several toxicity studies. It runs the risk of causing vitamin deficiencies when used in excess.

Dietary control: As used here, dietary control involves the manipulation of food allocations to maintain experimental animals on a pre-determined body weight growth curve. It can involve either dietary restriction of dietary supplementation depending on the individual animal and on the required growth curve.

Glucocorticoid: A steroid ligand of the glucocorticoid receptor, which evokes the glucocorticoid effect of raising blood glucose levels. Includes pharmaceuticals such as dexamethasone

Hypercorticism: Elevated secretion and blood concentrations of adrenal corticosteroids; predominantly corticosterone in rodents and cortisol in primates.

Nutrient stress: Hypoglycemia-induced stress resulting from reduced caloric intake, which can result from dietary restriction, short-term fasting or starvation.

Restraint stress: Experimental technique of producing a classic stress response in rodents by restricting their movements.

Weight-reduced mice: Mice which had lower body weight values and lower rates of growth due to either dietary restriction or exposure to a non-carcinogenic test chemical.

See reference 231 for more details. See also legends of Figures 1 and 2 for full names of hormones and signal transduction proteins .

The Authors

Dr. Julian Leakey earned his B.Sc. and Ph.D. degrees in the Department of Biochemistry at the University of Dundee, Scotland, U.K. He joined the Division of Reproductive and Developmental Toxicology at NCTR as a senior staff fellow in 1985. Between 1991 and 1997 he worked on the NCTR-NIA Project on Caloric Restriction. He is currently a member of NCTR’s Office of Scientific Coordination. He became a Diplomate of the American Board of Toxicology in 1995. His research interests include regulation of expression of drug metabolizing enzymes, effects of diet and obesity on inflammatory processes and carcinogenesis, and development and standardization of new animal models for use in chronic toxicity studies.

Dr. William Allaben is Associate Director for Scientific Coordination and the U.S. Food and Drug Administration’s (FDA) Liaison to National Toxicology Program (NTP), and as such directs the FDA’s participation in the NTP. Dr. Allaben received his Ph.D. in Physiology/ Pharmacology from Southern Illinois University and worked as a Research Fellow at the National Center for Toxicological Research (NCTR) before joining NCTR as a researcher in the Division of Carcinogenesis. Allaben is an Adjunct Professor in the Department of Toxicology and Pharmacology, University of Arkansas for Medical Sciences, Little Rock and an elected Fellow in the Academy of Toxicological Sciences. He has received numerous FDA recognition and honor awards including the Commissioner’s Special Citation/ Health Claims Task-force and the Award of Merit, FDA’s highest honor award. Dr. Allaben, with expertise in toxicology and carcinogenesis, has over 28 years experience conducting and/or managing regulatory research and testing programs.

John E. Seng is a Research Scientist/Study Director at Charles River Laboratories-Arkansas Division, Redfield, Arkansas. Dr. Seng received his Ph.D. in Interdisciplinary Toxicology from the University of Arkansas Medical Sciences in 1994 and worked as a National Toxicology Program Research Fellow (1994) and Study Director/Staff Fellow (1999) until joining Charles River Laboratories in 1999. During his tenure at NCTR, Dr. Seng's research focused on the refinement and standardization of new animal models for use in chronic toxicity studies and the influence of diet and obesity on detoxication pathways in the male reproductive system.

Regulatory Research Perspectives Editorial Board

Norris Alderson, Ph.D. – Office of the Commissioner (OC)
Daniel A. Casciano, Ph.D. – National Center for Toxicological Research (NCTR)
Thomas A. Cebula, Ph.D. – Center for Food Safety and Applied Nutrition (CFSAN)
Joanne N. Locke – Office of the Commissioner (OC)
Edward E. Max, Ph.D. – Center for Biologics Evaluation and Research (CBER)
Michael C. Olson – Office of Regulatory Affairs (ORA)
Mary S. Wolfe, Ph.D. – National Institute of Environmental Health Science (NIEHS)
Linda D. Youngman, Ph.D. – Center for Veterinary Medicine (CVM)
Hal Zenick , Ph.D. – Environmental Protection Agency (EPA)

DHHS/FDA/Jefferson Labs
National Center for Toxicological Research
3900 NCTR Road, HFT-1
Jefferson, Arkansas 72079-9502
Telephone: (870) 543-7516
Website: www.fda.gov/nctr

Editorial Matters:

Address for editorial matters noted above. Article may be republished without permission. Credit to Regulatory Research Perspectives as the source is appreciated.
Editor: Lionel A. Poirier, Ph.D.
Managing Editor/Layout: Virginia B. Taylor Email: virginia.taylor@fda.hhs.gov.