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Although a causal role of genetic alterations in human cancer is well established, it is still unclear whether dietary fat can modulate cancer risk in a predisposed population. Epidemiological studies suggest that diets rich in omega-3 polyunsaturated fatty acids reduce cancer incidence. To determine the influence of fatty acids on prostate cancer risk in animals with a defined genetic lesion, we used prostate-specific Pten-knockout mice, an immune-competent, orthotopic prostate cancer model, and diets with defined polyunsaturated fatty acid levels. We found that omega-3 fatty acids reduced prostate tumor growth, slowed histopathological progression, and increased survival, whereas omega-6 fatty acids had opposite effects. Introducing an omega-3 desaturase, which converts omega-6 to omega-3 fatty acids, into the Pten-knockout mice reduced tumor growth similarly to the omega-3 diet. Tumors from mice on the omega-3 diet had lower proportions of phosphorylated Bad and higher apoptotic indexes compared with those from mice on omega-6 diet. Knockdown of Bad eliminated omega-3–induced cell death, and introduction of exogenous Bad restored the sensitivity to omega-3 fatty acids. Our data suggest that modulation of prostate cancer development by polyunsaturated fatty acids is mediated in part through Bad-dependent apoptosis. This study highlights the importance of gene-diet interactions in prostate cancer.
A causal role of genetic alterations in human cancer is well established; however, environmental influence on cancer risk is not clearly understood. Over 2 decades, epidemiologic studies have been reported on the effect of dietary fat on prostate cancer risk (1). However, the mechanistic role of dietary fat in prostate cancer remains ill defined. Prostate cancer is the most frequently diagnosed cancer and a leading cause of cancer death in men in the US. There is a wide variation in international prostate cancer mortality rates; these are particularly high in Northern Europe and North America and much lower in Japan and other Asian countries (2). Yet small, latent carcinomas of the prostate diagnosed at autopsy are as common in Asian countries as in Western countries (3). Immigrants from Poland and Japan exhibit a significant increase in the risk of developing clinical prostate cancer when resident in the US (4–6). These findings implicate environmental variables, and possibly diet, as significant contributing factors.
Omega-3 and omega-6 polyunsaturated FAs (PUFAs) are essential FAs: mammals can neither synthesize them de novo nor interconvert them; therefore, they have to be taken in from diet. Many vegetable oils contain high levels of omega-6 PUFAs, whereas fish oil is a rich source of omega-3 PUFAs, mainly eicosapentaenoic acid (EPA; 20:5n-3) and docosahexaenoic acid (DHA; 22:6n-3). Diets with an omega-6/omega-3 PUFA ratio of 1 are recommended for human consumption by a panel of nutritionists (7), and diets with a similar ratio are consumed by some populations such as the Inuit (8). Current Western diets have omega-6/omega-3 ratios of approximately 30 (9), although they can be as high as 50 (10) (Supplemental Figure 1; supplemental material available online with this article; doi:10.1172/JCI31494DS1). Some evidence suggests that cyclooxygenase inhibitors, which block the metabolism of omega-6 PUFAs, are beneficial in prevention of colon (11) and prostate (12) cancer. However, the cardiovascular toxicity (13) of cyclooxygenase-2 inhibitors has jeopardized the clinical utility of these drugs. Reducing the intake of omega-6 PUFAs and increasing the proportion of dietary omega-3 is an attractive approach.
Inaccuracy in reporting dietary intake and difficulties in conducting mechanistic studies on human populations have hampered investigations on the role of dietary fat in prostate cancer development. Most experiments using animals have been performed in xenograft models and are limited by the fact that tumors grow at an ectopic site in an immune-deficient host environment. Moreover, dietary composition in animal diets is often poorly defined, and dietary intake is inadequately monitored. In an effort to overcome these limitations, we used prostate-specific Pten-knockout mice, an immune-competent, orthotopic prostate cancer model, and designed diets to investigate the influence of dietary PUFAs on prostate cancer risk in animals with this defined genetic lesion.
Mice with a defined genetic lesion, in this case loss of the tumor suppressor gene Pten, develop cancer spontaneously. To determine whether genetic cancer risk can be modified by dietary factors, wild-type mice and mice with Pten deletion were fed diets with different amounts of omega-3 and omega-6 fatty acids. Prostate-specific deletion of floxed Pten was achieved by expressing Cre recombinase under the control of a probasin promoter (PB). Mouse genotypes are PtenloxP/loxPPB-cre4–/– (wild-type), PtenloxP/+PB-cre4T/– (heterozygous), and PtenloxP/loxPPB-cre4T/– (homozygous). For simplicity, we hereafter refer to these mice as PtenP+/+, PtenP+/–, and PtenP–/–, respectively. Experimental diets included high–omega-3, low–omega-3, and high–omega-6 diets, with ratios of omega-6/omega-3 PUFAs of 1, 20, and 40, respectively. Diets were designed to be nutritionally balanced, with the same caloric input and percentage of energy from fat (Supplemental Table 1). Omega-6/omega-3 FA ratios in mouse blood and prostate tissues were similar to those in the respective diet (Supplemental Figure 2). In addition, phospholipid profiling demonstrated that approximately 5-fold more omega-3 PUFAs were incorporated at the sn-2 position in mice fed the high–omega-3 diet compared with mice fed with the low–omega-3 or the–high omega-6 diet (Supplemental Figure 2C). The 3 diets were absorbed equally well in mice of different genotypes at various ages and did not affect body weight (Supplemental Figure 3).
Mice were sacrificed at 5, 8, 12, and 24 weeks of age. After recording mouse body weight, we dissected, photographed, and weighed the anterior, dorsolateral, and ventral prostate (AP, DL, and VP) lobes. In the PtenP+/+ and PtenP+/– groups, the relative prostate weight (expressed as mg/25 g body weight) increased from approximately 29 to approximately 35 between 5 and 8 weeks and remained constant thereafter (Figure (Figure1).1). Diets did not affect the weight or gross appearance of these wild-type prostates. By contrast, the average prostate weight of PtenP–/– mice was significantly higher than that of PtenP+/+ or PtenP+/– mice starting at 8 weeks of age (Figure (Figure1).1). Remarkably, the prostate weight gain from 5 to 24 weeks was significantly less in mice fed the high–omega-3 diet compared with mice fed the high–omega-6 diet, with intermediary gains for mice on the low–omega-3 diet (Figure (Figure1).1). Age, treatment, and age/treatment interactions were all statistically significant (treatment, P < 0.001; age, P < 0.001; interaction, P = 0.018).
Prostate lobes from PtenP+/+ and PtenP+/– mice appeared morphologically normal at 5–24 weeks of age, regardless of diet. However, prostate lobes from PtenP–/– mice were clearly enlarged and showed increased vascularity as well as cellularity (Figure (Figure2A).2A). Pathological evaluation was performed to determine the presence of hyperplasia, carcinoma in situ (CIS), and invasive carcinoma in AP, DL, and VP lobes of PtenP–/– mice (Figure (Figure2,2, B and C, and Supplemental Figure 4). DL lobes developed a greater proportion of advanced lesions as compared with AP and VP lobes. Prostates from 8-week-old mice on the high–omega-3 diet were more likely to have normal or benign histology. For instance, all VP lobes from 8-week-old mice on the high–omega-3 diet were either normal or hyperplastic, whereas VP lobes from mice on the high–omega-6 diet frequently contained CIS and invasive carcinoma. Even in the DL lobe, where Pten deletion occurs earliest, only half of the mice fed the high–omega-3 diet developed invasive carcinoma, whereas 80% of mice fed the high–omega-6 diet had invasive carcinoma. Mice fed the low–omega-3 diet generally developed prostate lesions with intermediate histopathology.
It is noteworthy that omega-3 PUFAs slowed the histological progression of prostate tumors in 5- to 8-week-old PtenP–/– mice. Once carcinoma developed, omega-3 PUFAs induced apoptosis and decreased the growth of tumor mass. The probasin promoter, which drives the prostate-specific expression of cre, is activated by androgens. Levels of sex hormones increase in male mice around 6 weeks of age, resulting in efficient Pten deletion. Activity of the probasin promoter is highest in the lateral prostate followed by anterior and ventral lobes. Accordingly, invasive carcinoma developed earlier in the DL than the VP and AP lobes. To determine whether diets affected the Pten deletion rate, which may account for the difference in prostate cancer progression, we used 3 different approaches: (a) real-time quantification of the inactive Pten allele (Figure (Figure3,3, A and B); (b) enzymatic assay of a lacZ gene whose expression depends upon Cre activity (Figure (Figure3C);3C); and (c) Western blotting of the active form of Akt, which is indicative of Pten inactivation (Figure (Figure3C).3C). Our data showed a similar Pten deletion rate in mice on the high–omega-3 diet and the high–omega-6 diet, indicating that this was not a factor in the rate of cancer development.
Although dietary ingredients were carefully formulated, the diets necessarily included other fats besides the omega-3 and -6 PUFAs to keep the energy from fat constant (Supplemental Table 1). To eliminate these possible confounding effects, the fat1 transgene (14), encoding an omega-3 desaturase from Caenorhabditis elegans that converts omega-6 into omega-3 FAs, was bred into the prostate-specific Pten-knockout genetic background. PtenP–/– mice with or without the fat1 transgene (fat1T/– and fat1–/–, respectively) were both fed the high–omega-6 diet. Mice were sacrificed at 12 weeks of age, and prostates were dissected and weighed. The average omega-6/omega-3 ratio in the blood and prostate tissues of fat1T/– mice was 5, compared with 40 in fat1–/– mice (Table (Table1).1). Thus, fat-1 was able to convert most of the omega-6 PUFAs to omega-3. Relative prostate weights were significantly lower in PtenP–/–fat1T/– than that in PtenP–/–fat1–/– mice (Figure (Figure4;4; P < 0.006, Student’s t test). This genetic approach confirms the suppressive effect of omega-3 PUFAs on tumor growth observed with diet manipulation. Thus, the fat1 mouse results are consistent with our conclusion that omega-3 and omega-6 FAs have opposite effects on tumor growth.
Overall survival was also monitored for mice on the 3 different diets. PtenP+/+ mice remained free of tumors and had a survival rate of 100% within the time period monitored, regardless of diet. PtenP+/– mice also had a survival rate of 100%, although some prostates from mice on the high–omega-6 diet were hyperplastic or neoplastic. By contrast, the 12-month survival rate for PtenP–/– mice was 60% on the high–omega-3 diet, 10% on the low–omega-3 diet, and 0% on the high–omega-6 diet (Figure (Figure5).5). In fact, no PtenP–/– mice on the high omega-6 diet survived beyond 10 months of age in our experimental group. The main cause of death was bladder obstruction due to the prostate tumor compressing the urethra. Bladders were visibly dilated in some mice, and a few were even ruptured. These severe cases led to early death. For PtenP–/– mice that survived 6 months or longer, retention of urine in the AP lobes was consistently seen and often accompanied by pyelonephritis. Cox proportional hazards model analysis revealed that diets exerted statistically significant effects on survival (P = 0.005). Compared with the high–omega-6 diet, the high–omega-3 diet significantly increased the survival of PtenP–/– mice (hazard ratio 0.137; P = 0.0016), and, although to a lesser degree, the low–omega-3 diet significantly increased the survival as well (hazard ratio 0.337; P = 0.0338).
Pten encodes a phosphatidylinositol phosphatase that negatively regulates the PI3K/Akt signaling pathway. Akt promotes cell survival, protein synthesis, and proliferation when it is activated after being recruited to the plasma membrane by PI(3,4,5)P3 (phosphatidylinositol [3,4,5] triphosphate). Pten converts PI(3,4,5)P3 to PI(4,5)P2, resulting in lower activity of Akt. Loss of Pten is expected to increase Akt activity; therefore, we examined the status of Akt and its downstream signaling effectors in prostate samples of wild-type and Pten-knockout mice on the high–omega-3 and high–omega-6 diets.
The ratio of active (pSer473) Akt to total Akt protein was approximately 3- to 7-fold higher in prostates from the PtenP–/– mice than those from the PtenP+/+ mice. However, there was no significant difference in the active/total Akt ratio between PtenP–/– prostates from mice on the high–omega-3 and high–omega-6 diet (Figure (Figure6A).6A). Among the Akt effectors, the proapoptotic protein Bad was detected at higher levels in PtenP–/– than in PtenP+/+ prostates from mice on the high–omega-3 diet but not on the high–omega-6 diet. Additionally, the ratio of phosphorylated (pSer112) to total Bad was significantly lower in PtenP–/– prostates from mice on the omega-3 diet compared to the omega-6 diet (Figure (Figure6A).6A). Phosphorylation of Bad inhibits its proapoptotic function. Therefore, in mice on the omega-3 diet, the elevated Bad levels combined with a lower fraction of phosphorylated Bad would favor apoptosis. Indeed, a higher number of apoptotic cells was seen in PtenP–/– prostates from mice on the high–omega-3 than on the high–omega-6 diet as determined by immunohistochemistry of cleaved caspase-3 (Figure (Figure6B6B and Table Table2).2). Other Akt substrates, namely Foxo1 and Foxo3a and p70S6K (product of the gene Rps6kb1), were phosphorylated to similar degrees in PtenP–/– prostates regardless of diet (Supplemental Figure 5).
Omega-3 PUFA treatment inhibits tumor cell proliferation and induces apoptosis in culture (15). Since in vivo data suggest that omega-3 PUFAs may induce apoptosis through regulation of Bad, we further investigated the role of Bad in omega-3 PUFA–induced cell death. PC3 and LNCaP cells were mock infected or infected with lentiviruses expressing scrambled or Bad-specific short hairpin RNA (shRNA) (Figure (Figure7A).7A). Successful knockdown of Bad was confirmed by Western blotting (Figure (Figure7A).7A). These cells were then incubated with omega-3 or -6 PUFAs for 6 days, and the total cell number as well as the number of dead cells were determined by trypan blue exclusion. As shown in Figure Figure7B,7B, in mock- or scrambled shRNA–infected cells, omega-3 PUFA treatment increased the percentage of dead cells, whereas omega-6 PUFA treatment had no significant effect. Strikingly, knockdown of Bad completely eliminated omega-3 PUFA–induced cell death, and the percentage of dead cells was similar to that in untreated cells. By contrast, knockdown of Bad had little effect on omega-6 PUFA–treated cells. To confirm the specificity of the Bad knockdown construct, we introduced mouse Bad cDNA, which cannot be silenced by our shRNA designed to target human Bad. Introduction of Bad cDNA restored prostate cancer cell sensitivity to omega-3–induced cell death but did not significantly increase cell death upon omega-6 treatment (Figure (Figure7C).7C). These results suggest that cell death induced by omega-3 PUFAs is dependent on Bad expression.
Although a causal role of genetic alterations in human cancer is well established, epigenetic effects on cancer were not appreciated until recently (16). On the one hand, methylation, acetylation, and other molecular mechanisms implicated in epigenetics are being studied intensively (17, 18), but environmental factors causing these changes are largely unknown. On the other hand, factors such as diet are believed to affect cancer incidence, but molecular mechanisms have not been delineated. Here, we demonstrated the influence of defined dietary factors (omega-3 and -6 essential FAs) on a mouse model of prostate cancer with a known genetic risk (Pten deletion) and investigated underlying molecular mechanisms.
Epidemiological studies suggest that consumption of fish or fish oil reduces prostate cancer incidence (19, 20). One of the largest prospective studies, involving 6,272 men with 30 years of follow-up, indicated that fatty fish consumption was associated with decreased risk of prostate cancer (20). Serum levels of omega-3 PUFAs were reported to be significantly lower in patients with benign prostate hyperplasia and prostate cancer, and omega-6 PUFA levels were higher in patients with prostate cancer compared with age-matched controls (21). In prostate tissues, the percentage of total PUFAs was shown to be significantly lower in the presence of perineural invasion, seminal vesicle involvement, and stage T3 tumor. Levels of α linolenic acid (αLNA) omega-3 PUFAs were significantly lower when tumor extended to an anatomical or surgical margin. Total omega-3 levels and omega-3/omega-6 PUFA ratios were 1.5- to 3.3-fold lower in cases than in controls (22). In a 12-year prospective study of 47,882 men participating in the Health Professionals Follow-up Study, higher consumption of fish was strongly associated with a reduced risk of metastatic prostate cancer (23).
Nevertheless, molecular mechanisms of omega-3 PUFA effects on prostate cancer remain elusive. Our data show that the high–omega-3 diet, with an omega-6/omega-3 ratio recommended by nutritionists, could effectively deliver omega-3 PUFA to the prostate (Supplemental Figure 2), delay tumor formation (Figure (Figure1)1) and progression (Figure (Figure2),2), and prolong survival (Figure (Figure5)5) as compared with the high–omega-6 diet. Mice on the low–omega-3 diet, with an omega-6/omega-3 ratio of 20 as compared with a ratio of 1 in the high–omega-3 diet, showed intermediary tumor growth, progression, and survival. Therefore, the omega-6/omega-3 ratio appears to be a critical factor in the effectiveness of prostate cancer suppression, with a higher proportion of omega-3 being more effective. However, the absolute amount of PUFAs may also be of consequence, since high total fat intake has been associated with cancer incidence (24). In the present study, all diets contained 13% fat with 30% energy from fat, mimicking the average Western diet, which is relatively high in fat. The development of normal prostate was not affected by the ratio of omega-6 to omega-3 in the Pten wild-type background. This demonstrates the importance of gene-diet interactions and that genetic cancer risk can be modified favorably by omega-3 PUFAs. It remains to be determined whether there is a critical omega-6/omega-3 ratio threshold for achieving maximal tumor suppression. Clinically, prostate cancer is usually diagnosed in men age 60 or older, and cancer cells proliferate slowly. Therefore, dietary and/or chemoprevention are of particular importance for the management of prostate cancer. Our data imply a beneficial effect of omega-3 PUFAs on delaying the onset of human prostate cancer. It will be interesting to determine whether any beneficial effects can also be achieved by supplementing the diet with omega-3 PUFAs after tumor initiation has occurred.
Lipid signaling plays a critical role in cancer of the prostate and many other human cancers. The Pten tumor suppressor gene is the most frequently mutated gene in metastases of prostate cancer (25, 26). A significant loss of Pten expression is also seen in prostate tumor tissues (27). Homozygous deletion of Pten in mouse prostate results in prostate cancer development and metastasis (28). In addition, the PI3K pathway appears to be a dominant growth factor–activated cell survival pathway in LNCaP prostate carcinoma cells (29). It was shown that PI3K/Akt stimulates the androgen pathway (30, 31), which further highlights the importance of lipid signaling in prostate cancer.
We showed that the high–omega-3 PUFA diet reduced phosphorylation of the downstream Akt target Bad and increased tumor cell death compared with the high–omega-6 PUFA diet in PtenP–/– mice (Figure (Figure6).6). Knockdown of Bad in prostate cancer cells reduced the percentage of dead cells upon omega-3 PUFA treatment to baseline levels (Figure (Figure7B),7B), and introduction of exogenous Bad restored the phenotype (Figure (Figure7C).7C). It is well documented that phospho-Bad protein is sequestered by 14-3-3 and that dephosphorylation allows Bad to interact with antiapoptotic proteins Bcl-2 and/or Bcl-xL, thereby increasing the Bax/Bcl-2 ratio and favoring apoptosis (32). Expression of a nonphosphorylatable form of Bad induces apoptosis in various cell lines, including prostate cancer cells (33–35). Why is the Bad protein differentially phosphorylated in tumors from mice on omega-3 and omega-6 diet? Preliminary data indicated that in PtenP–/– prostates from mice on the omega-6 diet, a large proportion of active Akt was localized to the plasma membrane, whereas on the omega-3 diet, active Akt tended to be distributed through the cytoplasm. The pattern of PI(3,4,5)P3 localization coincided with that of the active Akt protein. The Akt kinase is activated by phosphoinositide binding (36, 37). In mammals, the sn-1 position on the glycerol backbone of phospholipids, including phosphoinositides, is usually linked to a saturated FA such as stearic acid and the sn-2 position often to an omega-6 PUFA such as arachidonic acid. Feeding cells or animals with omega-3 PUFAs results in replacement of omega-6 with omega-3 FAs at the sn-2 position (38), which was verified in the blood and prostate tissue of our experimental mice (Supplemental Figure 2C). Therefore, it is possible that incorporation of omega-3 PUFAs into phospholipids could alter the localization of both PI(3,4,5)P3 and the active form of Akt protein, resulting in differential Bad phosphorylation. On the other hand, it is also possible that this differential Bad phosphorylation is caused by a phosphatase. However, the nature of the enzymes involved in Bad dephosphorylation is somewhat controversial. Calcineurin and protein phosphatase 2A have been shown to dephosphorylate Bad in different cell types (39, 40). Experiments exploring the mechanism of Bad dephosphorylation in our system are ongoing.
We believe Bad-dependent modulation of apoptosis by omega-3 PUFAs to be a novel finding that could account, at least in part, for the proposed tumor-preventive properties of these FAs. In addition, omega-3 and -6 PUFAs can be metabolized by cyclooxygenases and lipoxygenases (41), and the resulting eicosanoids have different biological functions in processes such as proliferation, inflammation, and angiogenesis. These processes may contribute to carcinogenesis directly or indirectly. Indeed, we have noticed a reduction in microvessel density as well as CD3+ lymphocyte levels in tumors from mice fed the omega-3 diet compared with those fed the high–omega-6 diet. The significance of these changes in relation to the suppression of prostate cancer by omega-3 PUFAs is currently under investigation.
Prostate-specific Pten-knockout mice were generated by crossing PtenloxP/loxP mice (42) with mice of the ARR2Probasin-cre transgenic line PB-cre4, wherein the Cre recombinase is under the control of a modified rat prostate-specific probasin promoter (43), as previously reported (44). B6.129S4-Gt(ROSA)26Sortm1Sor/J mice, which have a floxed lacZ gene targeted to the ROSA26 locus, whose expression depends on Cre activity, were purchased from The Jackson Laboratory. For simplicity, PtenloxP/loxPPB-cre4–/– and PtenloxP/+PB-cre4–/– are referred to as PtenP+/+; PtenloxP/+PB-cre4T/– as PtenP+/–; PtenloxP/loxPPB-cre4T/– as PtenP–/–; and B6.129S4-Gt(ROSA)26Sortm1Sor/J as ROSA26LZ/LZ. F1 and F2 mice were maintained on experimental diets, and only F2 males were used in our experiments.
fat1-transgenic mice (14) were crossed with prostate-specific Pten-knockout mice. PtenP–/–fat1T/– and PtenP–/–fat1–/– mice were used in this study.
The PB-cre4, ROSA26LZ/LZ, and fat1 transgenic mice were of a congenic C57BL/6 background. They were backcrossed to C57BL/6 for more than 10 generations. The PtenloxP/loxP mice were of mixed C57BL/6 and BALB/c background. They were backcrossed to C57BL/6 for 3–5 generations.
Histopathological evaluation of mouse prostate tissues was performed by board-certified veterinary pathologists. The Bar Harbor classification system for scoring the benign and malignant growth in the prostates of genetically engineered mice was used (45). However, the authors prefer the term “carcinoma in situ” to “mPIN” (mouse prostatic intraepithelial neoplasia), as it accurately describes a preinvasive carcinoma lesion without requiring further clarification. Human PIN lesions, while being predictive of the development of an invasive adenocarcinoma, do not demonstrate direct invasion through the basement membrane into the surrounding stroma as the neoplastic epithelial lesions were seen to do in these transgenic mouse prostate glands.
All animals were maintained in an isolated environment in barrier cages and fed the specified diet. Animal care was conducted in compliance with the state and federal Animal Welfare Acts and the standards and policies of the US Department of Health and Human Services. The protocol was approved by our Institutional Animal Care and Use Committee at Wake Forest University.
Diets were prepared by the custom animal diet laboratory of the Animal Resources Program at Wake Forest University. All 3 diets contained 397 kcal/100 g, and 30% of energy was from fat, 50% from carbohydrates, and 30% from proteins. The omega-6/omega-3 ratio was 1 in the high–omega-3 diet, 20 in the low–omega-3 diet, and 40 in the high–omega-6 diet (Figure (Figure1B1B and Supplemental Table 1).
Prior to sacrifice of animals, approximately 200 μl of blood per mouse was collected through the retro-orbital vein, snap-frozen in liquid nitrogen, and stored at –80°C until analysis.
Total FAs were analyzed in the food, blood, and prostate of mice at the ages of 5, 8, and 12 weeks (5 mice per group). Internal standards, 1,2-dipentadecanoylglycero-3-phosphocholine and 1,2-didodecanoylglyceero-3-phosphoethanolamine, were added to each tube, and solvent was removed in a stream of Ar. The residue was dissolved in 1 ml of ethanol and then mixed with 10 μl of sample. Tissue was extracted using the method of Bligh and Dyer (46), with di-15:0 phosphatidylcholine (PC) or di-12:0 phosphatidylethanolamine (PE) as an internal standard. After extraction, the supernatant was decanted and saved. Protein pellets were saved for later analysis. Organic layers were combined and evaporated under a stream of Ar at 37°C then redissolved in 1 ml of ethanol. Sample preparation was based on the method of Metcalfe et al. (47) as used previously (48). The sample in ethanol was treated with 0.1 ml of 50% aqueous KOH, the tube was purged with Ar, and then heated to 60°C for 1 hour. After cooling, nonsaponifiable lipids were removed by extracting with 3 ml of hexane. The aqueous layer was acidified and extracted with 3 ml of hexane, and the hexane layer was removed and dried in a stream of Ar. The residue was treated with 0.5 M methanolic NaOH at 100°C for 5 minutes. After cooling, the sample was treated with 1 ml of 14% BF3 in methanol (Sigma-Aldrich), flushed with Ar, and then heated to 100°C for 5 minutes. After cooling, the samples were treated with 2 ml of hexane and 4 ml of saturated, aqueous NaCl. The hexane phase was transferred to a separate tube, dried in a stream of Ar, then diluted with hexane (500 μl for blood samples or 50 μl for tissue samples), and then 1 μl of solution was analyzed on a Trace MS interfaced to a Trace 2000 GC (Thermo Electron Corp.). Separation was accomplished using a 30 m × 0.25 mm diameter DB-WAX WCOT column (Agilent Technologies) with a 0.25-μm coating.
Tissue was extracted as described above and dissolved in 1 ml of CHCl3/MeOH (1:1, vol/vol). Blood was extracted by adding 10 μl of blood to 5 ml hexane/isopropanol (3:2, vol/vol) containing the internal standard d-15:0 PC or di-12:0 PE. After flushing the headspace with Ar and extracting for 1 hour at room temperature, the sample was centrifuged and supernatant decanted. Solvent was removed in a stream of Ar and sample redissolved in 1 ml of CHCl3/MeOH (1:1, vol/vol). Total phosphorus was analyzed using the method of Rouser et al. (49). Samples were diluted to 2 nmol/ml in CHCl3/MeOH (1:1, vol/vol) containing 1% formic acid for analysis and analyzed using a Quattro II electrospray triple quadrupole tandem mass spectrometer (Waters Corp.) as previously described (50). Precursor-ion analysis at 184 m/z in the positive ion mode identified PC molecular species. PE and phosphatidylserine (PS) molecular species were identified in the positive-ion mode by monitoring the common-neutral losses of 141 Da and 185 Da, respectively. The FA distribution of individual molecular species was determined in the negative-ion mode by product ion analysis of [M-CH3]-ions from PC, PE, or PS. The ion intensity of each spectrum was corrected for isotope effects and transmission losses.
The AP, DL, and VP lobes were dissected as described previously (44). Whole mouse and prostate were weighed. Prostate tissues were paraffin embedded for histology and immunohistochemistry, pulverized in liquid nitrogen for lipid analysis, homogenized in a buffer for Western blotting, or snap-frozen and OCT embedded for immunostaining of phosphoinositides.
A cohort of 90 mice (10 mice per group for PtenP+/+, PtenP+/–, and PtenP–/– mice on each of the 3 experimental diets) was followed for 12 months. Time to death was recorded. Death was either natural or by euthanasia (if mice were moribund), as recommended by veterinarians according to institutional policies.
Cleaved caspase-3 staining was performed with an anti–cleaved caspase-3 primary antibody (catalog 9661; Cell Signaling Technology), followed by a biotinylated anti-rabbit secondary antibody and streptavidin alkaline phosphatase (Super Sensitive Link-Label IHC Detection Systems; BioGenex), visualized with Vector Red Substrate (SK-5100; Vector Laboratories), and counterstained with hematoxylin. Representative whole prostate sections for omega-3– and omega-6–fed PtenP–/– mice were photographed in their entirety, and each VP, DL, and AP lobe was assembled by tiling individual images in Adobe Photoshop CS (Adobe Systems Inc.). The total number of epithelial cells was enumerated in all glands using Image-Pro Plus 4.5 software (Image Processing Solutions). Numbers of apoptotic cells were counted in every gland under a light microscope by 2 individuals. The apoptotic index for each prostate lobe was expressed as the number of apoptotic cells per thousand cells in tumor glands (glands with normal and hyperplastic morphology were excluded). Average apoptotic indices are presented.
Prostate tissues were homogenized or cells were lysed in a buffer (50 mM Tris-HCl pH 7.5, 150 mM NaCl, 0.5% NP-40, 1 mM DTT, 1 mM PMSF, 1× Protease Inhibitors [catalog 1697498; Roche Applied Science]) with phosphatase inhibitors (50 mM NaF, 1 mM Na3VO4, 50 mM β-glycerophosphate, and 40 mM p-nitrophenylphosphate). Western blotting was performed as described previously (51) with anti–pS437 Akt (catalog 3787), anti–total Akt (catalog 9272), anti–Bad pSer112 (catalog 9291), anti–total Bad (catalog 9292), anti–phosphorylated FoxO1 and -3a (catalog 9464), and anti–S6K pT389 (catalog 9205) antibodies (Cell Signaling Technology), as well as anti–β-actin (Sigma-Aldrich).
Prostate genomic DNA was extracted from 6-, 7-, and, 8-week-old PtenP–/– mice and diluted to final concentration of 100 ng/μl. Real-time PCR was performed for Pten lacking exon 5 and Il-2 (as a single copy number control) alleles using iCycler (Bio-Rad) with QuantiTect SYBR Green PCR kit (QIAGEN), using 100 ng genomic DNA per reaction. PCR reaction consisted of 50 cycles of 15 seconds at 94°C, 30 seconds at 57°C, and 45 seconds at 72°C. Reaction mixtures without genomic DNA were used as negative controls. Primers used were 5ι-TCCCAGAGTTCATACCAGGA-3ι and 5ι-GCAATGGCCAGTACTAGTGAAC-3ι for Pten Δ5; and 5ι-CTAGGCCACAGAATTGAAAGATCT-3ι and 5ι-GTAGGTGGAAATTCTAGCATCATCC-3ι for Il-2. For each primer set, a standard curve was constructed with dilutions of a reference genomic DNA sample. Three mice were used per data point, and each sample was analyzed in triplicate. Amounts of Pten Δ5 were normalized to Il-2, and average values were presented.
PtenloxP/loxPROSA26LZ/LZPB-cre4T/– mice were generated by crossing PtenL/+ROSA26LZ/+PB-cre4T/– males with PtenloxP/loxPROSA26LZ/LZ females. In these mice, the Cre recombinase is expressed in prostate epithelial cells under the control of the probasin promoter, and an inactive allele of the lacZ gene under ubiquitously active ROSA26 promoter. Cre-mediated recombination at loxP sites in the lacZ gene activated expression of catalytically active β-galactosidase (Figure (Figure3A),3A), whereas recombination at loxP sites in the Pten gene inactivated Pten. Prostate tissues from 6-week-old PtenloxP/loxPROSA26LZ/LZPB-cre4T/– mice were homogenized in Promega passive lysis buffer with 0.2 mM PMSF and 1 mM DTT. After 3 freeze-thaw cycles, tissue debris was removed by centrifugation at 16,000 g for 15 minutes. Protein concentration was measured with a Pierce BCA kit, and equal amounts of protein were assayed for β-galactosidase activity using Beta-Glo assay system (Promega). Briefly, 35 μl diluted sample was incubated with 35 μl Beta-Glo reagent for 45 minutes at room temperature. RLU were read on a TD-20120 luminometer (Turner Designs Inc.). Protein lysates from PtenloxP/loxPROSA26LZ/LZPB-cre4–/– mice were used as negative controls for background subtraction. Three mice per data point were used, and each sample was analyzed in duplicate. Averaged values with SEM are presented.
Portions of prostate tissues from the mice described above were snap frozen and OCT embedded. Sections (8-μm) were cut, fixed (2% formaldehyde, 0.2% glutaraldehyde in PBS) for 5 minutes. After 3 washes in PBS, sections were incubated in X-Gal staining solution (1 mg/ml X-Gal, 4 mM potassium ferricyanide, 4 mM potassium ferrocyanide, 2 mM magnesium chloride, 0.02% IGEPAL CA-630, 0.01% sodium deoxycholate) at 37κC for 2.5 hours. Finally, sections were washed in distilled water, counterstained with eosin, dehydrated, and mounted.
Protein lysates obtained as described above for the β-galactosidase activity assay were also used for Western blotting of pSer473 and total Akt as described in “Western blotting.”
To generate shRNA virus, Bad targeting sequence 5ι-GGCTTGGTCCCATCGGAAGttcaagagaCTTCCGATGGGACCAAGCC-3ι (human Bad sequence in capital letters and loop in italics) was cloned between the XhoI and HpaI sites into the pLL3.7 lentiviral vector, which has a GFP marker. A scrambled sequence 5ι-GGTACGGTCAGGCAGCTTCTttcaagagaAGAAGCTGCCTGACCGTACC-3ι was used as control. HEK293 cells were transfected with shRNA vector together with packaging vectors (VSVG, RSV-REV, and pMDLg/pRRE). Supernatants were collected 48 hours after transfection.
PC3, LNCaP, or LNCaP transfected with control vector and mouse Bad expression vector were used in knockdown experiments. Due to sequence variations, mouse cDNA is not susceptible to knockdown with our shRNA designed to target human Bad. G418-resistant colonies were isolated, verified for successful expression of the HA-tagged mouse Bad by Western blotting, and pooled. PC3, LNCaP, LNCaP (vector), and LNCaP (mBad) cells were infected with shRNA lentivirus expressing scrambled shRNA or Bad-specific shRNA or were mock infected for 2 days. Cells (10,000) were seeded in 6-well plates with 1 ml medium with or without 100 μg/ml LDL FAs (15). One milliliter of corresponding fresh medium was added every other day, and cells were incubated for a total of 6 days. Cells were enumerated by the trypan blue exclusion method. Cells were collected after counting and used for Western blotting of Bad and β-actin.
Mouse prostate weight data were analyzed using a 2-way ANOVA model. In these models, prostate weight adjusted for body weight (mg/25 g) was considered the outcome. The 2 factors of interest were treatment (mice were randomly assigned to each of the 3 groups: high–omega-3, low–omega-3, and high–omega-6) and age of mouse (4 levels: 5, 8, 12, and 24 weeks). In addition, the treatment-by-age interaction was examined in these models. The data was examined for assumptions of ANOVA modeling (homogeneity of variances, normality, etc.), and there did not appear to be any severe deviations. Significance testing was performed using 2-sided tests with α = 0.05 for all comparisons. For all ANOVA analyses, data for all mice were used (i.e., no mice needed to be excluded). Survival data were compared between treatment groups using Cox proportional hazards regression models. In these comparisons, 6 groups of mice had no events (all PtenP+/+ and PtenP+/– mice survived), so the inference was made based on the 3 PtenP–/– groups. Hazard ratios and P values were calculated using a 2-sided 0.05 α value to determine statistical significance. Pairwise comparisons were made between the high–omega-6 diet and the other 2 diets separately.
We are grateful to Bioriginal (Saskatoon, Saskatchewan, Canada), which generously provided omega-3 FAs used in this study. We thank Lingyi Lu (Department of Biostatistical Science) for statistical analysis and Karen Klein (Grant and Manuscript Development, Office of Research, Wake Forest University School of Medicine) for manuscript editing. This work was supported in part by NIH grants R01CA107668 and P01CA106742, the Chinese National Natural Science Foundation (no. 20576047), and the Chang Jiang Scholars Program.
Nonstandard abbreviations used: AP, anterior prostate; DL, dorsolateral prostate; PB, probasin promoter; PC, phosphatidylcholine; PE, phosphatidylethanolamine; PUFA, polyunsaturated FA; shRNA, short hairpin RNA; VP, ventral prostate.
Conflict of interest: The authors have declared that no conflict of interest exists.
Citation for this article: J. Clin. Invest. 117:1866–1875 (2007). doi:10.1172/JCI31494