The aim of this study is to investigate the effect of chlorogenic acid (CA) on 3T3-L1 adipocytes and its mechanism action. CA at 1-25 μM showed no cytotoxicity to 3T3-L1 pre-adipocytes and 3T3-L1 adipocytes. CA significantly inhibited oil red O-stained material (OROSM) and intracellular triglyceride levels in 3T3-L1 adipocytes in a concentration-dependent manner. In addition, CA down-regulated the glycerol-3–phosphate dehydrogenase (GPDH) and peroxisome proliferator–activated receptor γ (PPARγ) activity. A real-time polymerase chain reaction revealed that CA inhibited the PPARγ, CCAAT/enhancer-binding protein alpha (C/EBPα), sterol regulatory element binding protein-1c (SREBP-1c), and fatty acid synthase (FAS) gene expression, which may in part account for anti-adipogenesis of CA. Thus, CA could act as a potential lipid lowering functional resource.
A WHO survey indicates that in 2020, worldwide obesity has nearly triple since 1975. Most of the world’s population live in countries where overweight and obesity kills more people than underweight 1. Obesity is a civilization-related medical problem, which increases the risk of a number of diseases, such as hypertension, cardiovascular diseases, diabetes, high blood cholesterol, malignant neoplasms, osteoporosis, cancers and sleep disorders 2. The fundamental cause of obesity or overweight is an energy imbalance between calories intake and expenditure. Overweight and obesity are preventable by choosing healthier foods and regular physical activity (WHO, 2020). Therefore, preventing, controlling and treating overweight and obesity have become important goals. Many studies have reported that some natural products and food components are able to prevent overweight and obesity. For example, djulis has been reported to be effective in the inhibition of adipogenesis in 3T3-L1 cell 3, and an in vivo study has shown that oral administration of djulis has beneficial effects on hyperlipidemia in obese mice 4. The phytochemicals such as betanin, rutin and kaempferol suppressed lipid accumulation due to reduced gene expression of PPARγ, C/EBPα and SREBP-1c 3. Also, some reports have noted that bioactive compounds, such as flavonoids, may cause an inhibition of adipogenesis and lipogenesis, and induction of lipolysis as well as apoptotic death of adipose cells 5. These findings imply that complementary and alternative therapies with functional biomaterials can regulate lipid metabolism and prevent overweight and obesity. Consequently, the investigations of natural products or bioactive compounds for preventing and treating overweightness and obesity have received a great deal of attention.
Chlorogenic acid (CA) is a family of ester formed between quinic acid and 1-4 trans-cinnamic acids, residues of certain trans-cinnanic acids, most commonly caffeic, ferulic, and p-coumaric acids 6. CA is found in the seeds and leaves of many dicotyledonous plants. Therefore, it has been extensively investigated and recognized to have numerous biological activities, such as antioxidant, antidiabetic, anti-inflammatory, anticancer, antineurodegenerative, antihypertensive, and antilipidemic activities 7. In addition, 5-caffeoylquinic acid decreasing obesity in high-fat-diet induced rats may be associated with up-regulation of PPARα expression and down-regulation of LXRα expression. Beside these, there has been little research on the effectiveness of CA in regulating lipid accumulation. Thus, the aim of this study is to investigate the inhibitory effect of chlorogenic acid on lipogenesis of 3T3-L1 adipocytes, and its action mechanism is also elucidated.
3T3-L1 cell (BCRC Number: 60159) was obtained from the Bioresource Collection and Research Center (BCRC, Food Industry Research and Development Institute, Hsinchu, Taiwan). Chlorogenic acid was obtained from the Alfa Aesar (Heysham, Lancashire United Kingdom). Oil red O solution, 3-isobutyl-1-methylxanthine, dexamethasone, and insulin were obtained from Sigma (St. Louis, MO, USA). The dye MTT (3-[4, 5-dimethylthiazol-2-yl]-2, 5-diphenyltetrazolium bromide) was purchased from PanReac AppliChem (Darmstadt, Germany). Dulbecco’s modified Eagle’s medium (DMEM), Trypsin-EDTA, penicillin-streptomycin, bovine calf serum, and fetal bovine serum were purchased from Gibco (Grand Island, NY, USA). Anti-PPAR and anti-α-actin were purchased from Cell Signaling Technology (Danvers, MA, USA). All other chemicals were reagent grade.
2.2. Cell Culture3T3-L1 preadipocytes were planted into 6-well plates and maintained in DMEM supplemented with 10% bovine calf serum at 37°C in a humidified 5% CO2 incubator. Adipocytic differentiation was induced by the differentiation medium A (0.5 mM 3-isobuty1-1-methylxanthine, 1 μM dexamethasone, 1 μM insulin, 1.5 g/L sodium bicarbonate, 10% fetal bovine serum and 1% antibiotic dissolved in high glucose DMEM) that were added to culture medium in every 48 h for 4 days. Afterwards, the medium was changed to differentiation medium B (1 μM insulin, 1.5 g/L sodium bicarbonate, 10% fetal bovine serum and 1% antibiotic dissolved in high glucose DMEM) and was freshly replaced every day. The cells were harvested 8 days after the initiation of differentiation. 3
2.3. Cell Viability AssayCell viability was assessed by the MTT viability assay 8. The culture media containing test samples (1-25 µM) was added to each well and the cells were incubated for 24 h, with untreated cells served as control. Then, culture media was replaced with MTT (0.5 mg/mL) and incubated in the dark for 1 h. Formazan crystals were solubilized (100% DMSO), and absorbance was measured using an ELISA reader (Thermo Multiskan GO, Waltham, MA, USA) at 550 nm.
2.4. Oil Red O-Staining of 3T3-L1 AdipocytesIntracellular lipid accumulation was measured using Oil red O 9. Freshly 60 mL Oil red O solution (0.5% in isopropanol) and 40 mL deionized water was prepared for the Oil red O working solution. Cells were incubated with test samples for 24 h at 37°C in a humidified 5% CO2 incubator. Cells were washed twice with phosphate buffered saline (PBS, pH 7.4) and then fixed with 10% neutral buffered formalin for at least 20 min at room temperature. After fixation, cells were washed twice with PBS and stained with the Oil red O working solution for 60 min. The image of stained cells was photographed, and then eluted stained Oil red O by adding 100% isopropanol, finally, the optical density was measured at 510 nm in ELISA reader (Thermo Multiskan GO).
2.5. Quantification of Intracellular TriglycerideCells were incubated with test samples for 24 h at 37°C in a humidified 5% CO2 incubator. Cells were collected and lysed in lysis buffer (1% Triton X-100 in PBS) for 30 min on ice box. The total triglyceride content in cells was determined using a commercial triglyceride assay kit (Cayman Chemical, Ann Arbor, MI, USA). The optical density of each well was determined at 550 nm using an ELISA reader (Thermo Multiskan GO). The protein concentration was estimated with the Pierce™ BCA protein assay kit (Thermo Scientific, Rockford, IL, USA) using bovine serum albumin as a standard. Inhibition (%) was expressed as percent decrease in triglyceride content against control (0%).
2.6. Determination of Glycerol-3-Phosphate Dehydrogenase Activity3T3-L1 adipocytes were harvested 8 days after the initiation of differentiation. Cells were incubated with 10-25 µM of test samples for 24 h at 37°C in a humidified 5% CO2 incubator. Cells were washed twice carefully with ice-cold PBS on 3T3-L1 adipocytes, and lysed in 25 mM Tris/1 mM EDTA, pH 7.5 for the measurement of glycerol-3-phosphate dehydrogenase (GPDH) specific activity. GPDH activity was determined by Glycerol-3-Phosphate Dehydrogenase Activity Colorimetric Assay Kit, (Biovision, Milpitas, CA, USA). The optical density of each well was determined at 450 nm using an ELISA reader (Thermo Multiskan GO). Protein concentration was determined by the Pierce™ BCA protein assay kit (Thermo Scientific) using bovine serum albumin as a standard. Enzyme activity was expressed as units of activity/mg protein. Inhibition (%) was expressed as percent decrease in GPDH activity against control (0%).
2.7. RNA Extraction and Real-Time PCRTotal RNA was extracted using Total RNA Isolation Kit (NA017-0100, GeneDireX, Las Vegas, NV, USA) according to the manufacturer’s instructions. RNA quantity and purity were checked by spectrophotometric analysis at 260 and 280 nm. One microgram of total RNA was reverse transcribed into cDNA using GScript First-Strand Synthesis Kit (MB305-0050, GeneDireX). The lists of specific primers (Invitrogen, Carlsbad, CA, USA) were: GAPDH, Forward: 5′GTATGACTCCACTCACGGCAAA-3′ (N3541G11), Reverse:5′-GGTCTCGCTCCTGGAAGATG-3′ (N3541H01); PPARγ, Forward: 5′-TTTTCAAGGGTGCCAGTTTCGATCC-3′ (N3541H02), Reverse: 5′-AATCCTTGGCCCTCTGAGAT-3′ (N3541H03); C/EBPα, Forward: 5′-CGCAAGAGCCGAGATAAAGC-3′ (N3541G05), Reverse: 5′-CACGGCTCAGCTGTTCCA-3′(N3541G06); Sterol regulatory element binding protein 1c (SREBP/lc), Forward: 5′-GGAGCCATGGATTGCACAT-3′ (N3541H06), Reverse: 5′-GCTTCCAGAGAGGAGGCCAG-3′ (N3541H07); FAS, Forward: 5′-TGGGTTCTAGCCAGCAGAGT-3′ (N3541G09), Reverse: 5′-TACCACCAGAGACCGTTATGC-3′ (N3541G10).
The primers were added at final concentration of 250 nM to a 20 μL reaction mixture containing 4 μL of 5× OmicsGreen qPCR Master Mix and 1 μL of DNA template (stock conc. 1 μg/mL). The PCR (StepOnePlus™ Real-Time PCR System, Applied Biosystems™, Foster, CA, USA) conditions were denaturation at 90°C for 15 s, annealing at 60–65°C for 20 s, and elongation at 72°C for 20 s in a cycle of 40 (OmicsGreen qPCR 5× Master Mix with ROX Dye, QE3931, Omics Bio, Taipei, Taiwan). The relative levels of gene expression were quantified using the ΔΔCt method, which results in a ratio of target gene expression relative to equally expressed housekeeping genes (GAPDH) 10.
2.8. Western Blot Analysis3T3-L1 adipocytes were harvested 8 days after the initiation of differentiation. Cells were incubated with 10-25 μM of test samples for 4 h at 37°C in a humidified 5% CO2 incubator. Cells were collected and lysed in ice-cold lysis buffer (20 mM Tris-HCl (pH 7.4), 2 mM EDTA, 500 μM sodium orthovanadate, 1% Triton X-100, 0.1% SDS, 10 mM NaF, 10 μg/mL leupeptin and 1 mM PMSF). The protein concentration was estimated with the PierceTM BCA protein assay kit (Thermo Scientific) using bovine serum albumin as a standard. Proteins were fractionated on a SDS-PAGE gel and blotted for 2.5 h at 100 V. The proteins in the gel were transferred to a PVDF membrane. The membrane was blocked with 5% BSA in PBST (0.1% v/v Tween-20 in PBS, pH 7.2) for 1 h. α-actin (1:1000 dilution) and PPARγ (1:1000 dilution) of primary antibodies were used in this study. Goat anti-rabbit IgG-HRP and rabbit anti-rabbit IgG-HRP (Jackson, West Grove, Chester, PA, USA) were used as secondary antibodies, and ECL Prime (Advansta Inc., Menlo Park, CA, USA) reagent was used for developing. Membranes were incubated with primary antibody at 4°C overnight and then with secondary antibody for 1 h. Membranes were washed in PBST for 10 min three times between each step. Blots were developed using the Western Bright ECL kit (Advansta Inc.), exposed to Gel Electrophoresis Documentation-Multi-function Gel Image system (Topbio Co., Taipei, Taiwan). The relative expression of proteins was quantified densitometrically using the Image J software (Wayne Rasband, Madison, WI, USA) and calculated according to the reference bands of α-actin 3.
2.9. Statistical AnalysisData are expressed as mean ± SD, and ANOVA was conducted by using the SPSS software (SPSS Inc., Chicago, IL, USA). When a significant F ratio was obtained (p < 0.05) a post hoc analysis was conducted between groups by using a Duncan’s multiple range tests or a Dunnett’s test. p-Values of less than 0.05 were considered statistically significant.
To study whether CA is able to induce cytotoxicity on 3T3-L1 cells, the cytotoxicity of CA was investigated using MTT assay. The effect of CA on cell growth in 3T3-L1 preadipocytes is shown in Figure 1A. The result indicated that CA at 1-25 µM exhibited no cytotoxicity to 3T3-L1 preadipocytes after 24 h of incubation with CA. Moreover, the 3T3-L1 cells were allowed to differentiate into adipocytes for 8 days, and then the mature cells were incubated for 72 h in medium with different concentrations of CA (1-25µM). As shown in Figure 1B, none of CA in the range from 1-25µM showed any cytotoxic effects on the viability of 3T3-L1 adipocytes. These results indicate that CA at 1-25µM does not affect 3T3-L1 preadipocyte viability and is not cytotoxic to 3T3-L1 adipocytes.
In this study, 3T3-L1 adipocytes undergoing induced differentiation were incubated with different concentrations of CA (10 and 25 µM). The effect of CA on adipogenesis was determined in relation to control cells. The level of accumulated lipid was analyzed in the culture after completion of the differentiation process. Figure 2 shows the effects of CA on lipid accumulation in 3T3-L1 adipocytes. The microscopic images of oil red O-stained adipocytes and the number of lipid droplets in the differentiated cells are shown in Figure 2A and 2B. Staining of lipid droplets with oil red O showed that their accumulation in cells exposed to CA was lower (Figure 2A). Meanwhile, lipid content in adipocytes was dependent on the CA dose (Figure 2B). Quantitatively, 25 µM CA reduced lipid accumulation by 28.0% in 3T3-L1 adipocytes. In addition, further determination of the effect of CA on the triglyceride level was done. Figure 2C shows the effect of CA on the triglyceride level in 3T3-L1 adipocytes. The addition of CA in the maturation medium caused a decrease in the triglyceride level. This reduction occurred in a dose-dependent manner, reaching a reduction of 19.6 and 21.7% for 10 and 25µM CA, respectively.
Glycerol-3-phosphate dehydrogenase (GDPH) catalyzes the formation glycerol-3-phosphate, and plays an essential role in glycerolipid metabolism 11. Therefore, it is regarded as a marker of adipogenesis. The present study examined the effect of CA on GPDH activity. As shown in Figure 3A, the intracellular GPDH activity was concentration-dependently inhibited in cells treated with CA. The cells treated with 25µM CA showed suppression of GPDH activity up to 18.0%, in comparison with control cells. In addition, PPARγ is a master regulator of adipocyte differential and metabolism. As shown in Figure 3B, in the CA-treated adipocytes, the PPARγ protein expression was decreased in a concentration-dependent manner. The results obtained indicate that CA has inhibitory activity on adipogenesis.
3.3. CA inhibits Adipocyte-Specific Gene ExpressionTo understand whether the suppressed increase in lipid accumulation and GPDH activity in adipocytes results from a CA-regulated alternation in the differentiation process, the expression of adipogenic genes was determined by quantitative real time RT-PCR. Figure 4 shows the effect of CA on expression of adipogenic genes in 3T3-L1 adipocytes. In the cells treated with CA at 10 and 25 µM, the mRNA levels of PPARγ, C/EBPα, SREBP-1c and FAS were determined after the induction of the differentiation process in 3T3-L1 adipocytes. The results show that CA inhibited the mRNA expression of PPARγ (Figure 4A), C/EBPα (Figure 4B), SREBP-1c (Figure 4C), and FAS (Figure 4D) in a dose-dependent manner, compared to the control cells. The mRNA expression levels of PPARγ, C/EBPα, SREBP-1c and FAS in 3T3-L1 adipocytes treated with 25µM CA decreased to 35%, 11 %, 36%, and 45%, respectively, of that of control cells. Consistent with the mRNA results, Western blot analyses revealed that CA markedly suppressed the protein expression levels of PPARγ (Figure 3B). That is to say, CA-associated attenuation of PPARγ gene expression was accompanied by a decrease in the corresponding proteins. These results indicate that CA is able to down-regulate the expression of adipogenic genes through an adipogenic process, thereby leading to inhibition of lipid accumulation in 3T3-L1 adipocytes.
It has been documented that at a molecular level, pre-adipocyte differentiation is regulated by PPARγ and C/EBPα, the down-stream targets of SREBP-1c. PPARγ, a ligand-activated transcriptional factor, is expressed predominantly in adipocytes and serves as the primary regulator of adipocyte differentiation 12. Moreover, PPARγ plays a pivotal role in inflammation and glucose metabolism 13. C/EBPα is a key transcriptional factor in adipogenesis and its expression is activated by C/EBPβ, C/EBPδ, and PPARγ in adipocytes, 3, 14. In other words, preadipocyte differentiation is regulated by PPARγ and C/EBPα. In addition, PPARγ and C/EBPα activate the expression of genes involved in adipogenesis, such as adipocyte protein 2 (aP2), lipoprotein lipase (LPL), fatty acid transporter, GlUTA, SCDI, and CD36, which mediate fatty acid or glucose uptake into adipocytes, triglyceride hydrolysis and lipogenesis 15, 16. Thereafter, adipocytes incorporate glucose and free fatty acid to synthesize and accumulate lipids as energy, resulting in an increase in cell size 16. SREBP-1c, a transcriptional factor, can stimulate genes related to de novo fatty-acid synthesis, such as FAS, ATP-citrate lyase (ACL), acetyl-CoA, carboxylase (ACC), stearoyl-CoA desaturase (SCP), and glyceraldehydes-3-phosphate acyltransferase (GPAT) 3, 17. As shown in Figure 4C, CA significantly reduced the mRNA levels of SREBP-1c, leading to prevention of SREBP-1c translocation to the nucleic acid, and finally inhibiting PPARγ, C/EBPα, and FAS expression. Many natural products and bioactive compounds with anti-adipogenic effect such as rutin, kaempferol and betanin were reported to inhibit adipogenesis due to suppression of these transcriptional factors 3. Figure 4 shows that CA down-regulated the expression of SREBP-1c and downstream target genes, PPARγ, C/EBPα, and FAS in differentiated cells. Thus, CA effectively suppressed lipid formation and adipogenesis by blocking adipogenic transcriptional factors.
AMPK, playing and important role in regulating lipids metabolism, glycogen breakdown, glycolysis, and glucose uptake, is a key sensor of fuel and energy status in skeletal muscles 18. The activation of AMPK leads to a decrease in the ACC activity, activation of malonyl CoA decarboxylase and reduction of the inhibitory effect of malonyl CoA to carnitine palmitoyl transterase-1, and further increases fatty acid oxidation 18. The amino-imidazole carboxamide ribonucleotide (AICAR), an activator of AMPK, was proven to inhibit 3T3-L1 adipocyte differentiation by suppressing the expression of SREBP-1, PPARγ, and C/EBPα 13. In other words, activation of AMPK causes the inhibition of adipogenesis. Although the influence of CA on the up-regulation of AMPK activation was not explored, the findings of Chen et al. 13 may support our results that CA up-regulates AMPK activation, resulting in inhibition of SREBP-1c, PPARγ, C/EBPα, and FAS expression during 3T3-L1 adipocyte differentiation.
CA, referred to an ester of caffeic acid and quinic acid, is present in a variety of edible plants. This phenolic phytochemical is known to have many biological activities. In addition, according to the results obtained, CA reduces the lipid accumulation by down-regulating the adipogenesis-related transcriptional factors, PPARγ, C/EBPα, SREBP-1c, and FAS during the differentiation process. These novel biological findings are helpful in understanding the antiadipogenic activity of CA. Considering the multiple biofunctional effects of CA, it may contribute to an inhibition of adverse metabolic effects connected with excessive growth of the adipose tissue.
In this study, the results show that CA inhibits adipogenesis by down-regulating the expression of PPARγ, C/EBPα, SREBP-1c and FAS. Consequently, the number of viable fully differentiated adipocytes is decreased, and lipid accumulation is limited. Therefore, CA with its anti-adipogenic effect, shows potential for development as an anti-obesity agent. However, further in vivo study is necessary to verify the anti-obesity activity of CA.
This research work was supported by research grants from Chi Mei Medical Center (CMFHR10510 and CMFHR10813).
The authors declare no conflict of interest.
| [1] | WHO, Obesity and overweight, 2020 https://www.who.int/news- room/fact-sheets/detail/obesity-and-overweight. | ||
| In article | |||
| [2] | Tzeng, T.F., Lu, H.J., Liou, S.S., Chang, C.J., Liu, I.M., “Reduction of lipid accumulation in white adipose tissues by Cassia tora (Leguminosae) seed extract is associated with AMPK activation”, Food Chem, 136, 1086-1094, 2013. | ||
| In article | View Article PubMed | ||
| [3] | Chyau, C.C., Chu, C.C., Chen, S.Y., Duh, P.D., “The inhibitory effects of djulis (Chenopodium formosanum) and its bioactive compounds on adipogenesis in 3T3-L1 adipocytes”, Molecules, 23(7), 1780, 2018. | ||
| In article | View Article PubMed | ||
| [4] | Chen, S.H., Chu, C.C., Lin, Y.C., Duh, P.D., “Djulis (Chenopodium formosanum) and its bioactive compounds for management of hyperlipidemia and hyperglycemia in high-fat diet-fed mice”, J Food Nutr Res, 7, 452-457, 2019. | ||
| In article | View Article | ||
| [5] | Kowalska, K., Olejnik, A., Rychlik, J., Graje, W., “Cranberries (Oxycoccus quadripetalus) inhibit adipogenesisand lipogenesis in 3T3-L1 cells”, Food Chem, 148, 246-252, 2014. | ||
| In article | View Article PubMed | ||
| [6] | Xu, J.G., Hu, Q.P., Liu, Y., “Antioxidant and DNA-protective activities of chlorogenic acid isomers”, J Agric. Food Chem, 60, 11625-11630, 2012. | ||
| In article | View Article PubMed | ||
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| In article | View Article PubMed | ||
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| In article | View Article PubMed | ||
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| In article | View Article PubMed | ||
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| In article | View Article PubMed | ||
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| In article | View Article PubMed | ||
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| In article | View Article PubMed | ||
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| In article | View Article PubMed | ||
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| In article | View Article PubMed | ||
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| In article | View Article PubMed | ||
| [16] | Ogawa, T., Tabata, H., Katsube, T., Ohta, Y., Shiwaku, K., “Suppressive effect of hot water extract of wasabi (Wasabia japonica Matsum.) leaves on the differentiation of 3T3-L1 preadipocytes”, Food Chem, 118, 239-244, 2010. | ||
| In article | View Article | ||
| [17] | Domínguez-Avila, J.A., Alvarez-Parrilla, E., López-Díaz, J.A., Maldonado-Mendoza, I.E., Gómez-García, M.D.C., de la Rosa, L.A., ”The pecan nut (Carya illinoinensis) and its oil and polyphenolic fractions differentially modulate lipid metabolism and the antioxidant enzyme activities in rats fed high-fat diets”, Food Chem, 168, 529-537, 2015. | ||
| In article | View Article PubMed | ||
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| In article | View Article PubMed | ||
Published with license by Science and Education Publishing, Copyright © 2020 Ching-Chih Liu, Jen-Yin Chen, Chin-Chen Chu, Shih-Ying Chen, Heuy-Ling Chu and Pin-Der Duh
This work is licensed under a Creative Commons Attribution 4.0 International License. To view a copy of this license, visit
https://creativecommons.org/licenses/by/4.0/
| [1] | WHO, Obesity and overweight, 2020 https://www.who.int/news- room/fact-sheets/detail/obesity-and-overweight. | ||
| In article | |||
| [2] | Tzeng, T.F., Lu, H.J., Liou, S.S., Chang, C.J., Liu, I.M., “Reduction of lipid accumulation in white adipose tissues by Cassia tora (Leguminosae) seed extract is associated with AMPK activation”, Food Chem, 136, 1086-1094, 2013. | ||
| In article | View Article PubMed | ||
| [3] | Chyau, C.C., Chu, C.C., Chen, S.Y., Duh, P.D., “The inhibitory effects of djulis (Chenopodium formosanum) and its bioactive compounds on adipogenesis in 3T3-L1 adipocytes”, Molecules, 23(7), 1780, 2018. | ||
| In article | View Article PubMed | ||
| [4] | Chen, S.H., Chu, C.C., Lin, Y.C., Duh, P.D., “Djulis (Chenopodium formosanum) and its bioactive compounds for management of hyperlipidemia and hyperglycemia in high-fat diet-fed mice”, J Food Nutr Res, 7, 452-457, 2019. | ||
| In article | View Article | ||
| [5] | Kowalska, K., Olejnik, A., Rychlik, J., Graje, W., “Cranberries (Oxycoccus quadripetalus) inhibit adipogenesisand lipogenesis in 3T3-L1 cells”, Food Chem, 148, 246-252, 2014. | ||
| In article | View Article PubMed | ||
| [6] | Xu, J.G., Hu, Q.P., Liu, Y., “Antioxidant and DNA-protective activities of chlorogenic acid isomers”, J Agric. Food Chem, 60, 11625-11630, 2012. | ||
| In article | View Article PubMed | ||
| [7] | Limwachiranon, J., Huang, H., Li, L., Lin, X., Zou, L., Liu, J., Zou, Y., Aalim, H., Duan, Z., Luo, Z., “Enhancing stability and bioaccessibility of chlorogenic acid using complexation with amylopectin: A comprehensive evaluation of complex formation, properties, and characteristics”, Food Chem, 311, 125879, 2020. | ||
| In article | View Article PubMed | ||
| [8] | Hsu, C.L., Yen G.C., “Effects of flavonoids and phenolic acids on the inhibition of adipogenesis in 3T3-L1 adipocytes”, J Agric Food Chem, 55(21), 8404-8410, 2007. | ||
| In article | View Article PubMed | ||
| [9] | Tzeng, T.F., Liu, I.M., “6-gingerol prevents adipogenesis and the accumulation of cytoplasmic lipid droplets in 3T3-L1 cells”, Phytomedicine, 20(6), 481-487, 2013. | ||
| In article | View Article PubMed | ||
| [10] | Noh, J.R., Kim, Y.H., Hwang, J.H., Gang, G.T., Yeo, S.H., Kim, K.S., Oh, W.K., Ly, S.Y., Lee, I.K., Lee, C.H.,” Scoparone inhibits adipocyte differentiation through down-regulation of peroxisome proliferators-activated receptor γ in 3T3-L1 preadipocytes”, Food Chem, 141(2),723-730. 2013. | ||
| In article | View Article PubMed | ||
| [11] | Zhao, Y., Li, X., Wang, F., Zhao, X., Gao, Y., Zhao, C., He, L., Zuotong Li, Z., Xu, J., “Glycerol-3-phosphate dehydrogenase (GPDH) gene family in Zea mays L.: Identification, subcellular localization, and transcriptional responses to abiotic stresses”, PLOS ONE. 2018. | ||
| In article | View Article PubMed | ||
| [12] | Tan, X.C., Chua, K.H., Ram, M.R., Kuppusamy, U.R., “Monoterpenes: Novel insights into their biological effects and roles on glucose uptake and lipid metabolism in 3T3-L1 adipocytes”, Food Chem, 196, 242-250, 2016. | ||
| In article | View Article PubMed | ||
| [13] | Chen, Y.Y., Lee, M.H., Hsu, C.C., Wei, C.L., Tsai, Y.C. “Methyl cinnamate inhibits adipocyte differentiation via activation of the CaMKK2–AMPK pathway in 3T3-L1 preadipocytes”, J Agric Food Chem, 60, 4, 955-963, 2012. | ||
| In article | View Article PubMed | ||
| [14] | Fujimori, K.; Shibano, M., “Avicularin, a plant flavonoid, suppresses lipid accumulation through repression of C/EBPalpha-activated GLUT4-mediated glucose uptake in 3T3-L1 cells”, J Agric Food Chem, 61, 5139-5147, 2013. | ||
| In article | View Article PubMed | ||
| [15] | Kowalska, K., Olejnik, A., Rychlik, J., Grajek, W., “Cranberries (Oxycoccus quadripetalus) inhibit adipogenesis and lipogenesis in 3T3-L1 cells”, Food Chem, 148, 246-252, 2016. | ||
| In article | View Article PubMed | ||
| [16] | Ogawa, T., Tabata, H., Katsube, T., Ohta, Y., Shiwaku, K., “Suppressive effect of hot water extract of wasabi (Wasabia japonica Matsum.) leaves on the differentiation of 3T3-L1 preadipocytes”, Food Chem, 118, 239-244, 2010. | ||
| In article | View Article | ||
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