Plac8 belongs to an evolutionary conserved family of proteins, mostly abundant in plants where they control fruit weight through regulation of cell number. In mice, Plac8 is expressed both in white and brown adipose tissues and we previously showed that Plac8−/− mice develop late-onset obesity, with abnormal brown fat differentiation and reduced thermogenic capacity. We also showed that in brown adipocytes, Plac8 is an upstream regulator of C/EBPβ expression. Here, we first assessed the role of Plac8 in white adipogenesis in vitro. We show that Plac8 is induced early after induction of 3T3-L1 adipocytes differentiation, a process that is prevented by Plac8 knockdown; similarly, embryonic fibroblasts obtained from Plac8 knockout mice failed to form adipocytes upon stimulation of differentiation. Knockdown of Plac8 in 3T3-L1 was associated with reduced expression of C/EBPβ, Krox20, and Klf4, early regulators of the white adipogenic program, and we show that Plac8 could transactivate the C/EBPβ promoter. In vivo, we show that absence of Plac8 led to increased white fat mass with enlarged adipocytes but reduced total number of adipocytes. Finally, even though Plac8−/− mice showed impaired thermogenesis due to brown fat dysfunction, this was not associated with changes in glycemia or plasma free fatty acid and triglyceride levels. Collectively, these data indicate that Plac8 is an upstream regulator of C/EBPβ required for adipogenesis in vitro. However, in vivo, Plac8 is dispensable for the differentiation of white adipocytes with preserved fat storage capacity but is required for normal fat cell number regulation.
Citation:Jimenez-Preitner M, Berney X, Thorens B (2012) Plac8 is required for White Adipocyte Differentiation in vitro and Cell Number Control in vivo. PLoS ONE 7(11): e48767. doi:10.1371/journal.pone.0048767
Editor: Giorgio Sesti, Universita Magna-Graecia di Catanzaro, Italy
Received: May 24, 2012; Accepted: October 5, 2012; Published: November 14, 2012
Copyright: © 2012 Jimenez-Preitner et al. This is an open-access article distributed under the terms of the Creative Commons Attribution License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original author and source are credited.
Funding:Swiss National Foundation grants No. 31003A-120472 to MJP and 3100A0-113525 to BT. (http://www.snf.ch/)and by the European Union Sixth Framework Program on Hepatic and Adipose Tissue and Functions in the Metabolic Syndrome (EU-FP6 HEPADIP, http://www.hepadip.org/) to BT. The funders had no role in study design, data collection and analysis, decision to publish, or preparation of the manuscript.
Competing interests: The authors have declared that no competing interests exist.
Adipogenesis is the process by which fibroblastic-like preadipocytes differentiate into adipocytes capable of storing fat in the form of triglycerides , . In vivo, white adipocytes store triglycerides in a single large lipid droplet from which free fatty acids can be released during the fasted state and secreted in the blood to provide metabolic energy to other tissues, such as muscle and liver. Imbalance between fat storage and release by adipocytes may lead to gain or loss of body weight. In obesity, excess fat storage and adipocyte enlargement are often associated with local inflammation and insulin resistance, production of cytokines, which can propagate insulin resistance to other tissues, and exaggerated lipolysis causing storage of fat in liver, muscles, or pancreatic beta-cells , , .
Understanding the molecular pathways controlling adipocytes differentiation from precursor cells is therefore important as this knowledge may help control adipocyte number and fat mass. A large body of research has identified a transcriptional cascade regulating white and brown fat differentiation. Common mechanisms controlling the differentiation of both types of fat tissues include activation of the CAAT/Enhancer Binding Protein ß (C/EBPβ), which activates C/EBPα and C/EBPδ; these transcription factors then stimulate expression of peroxisome proliferator-activated receptor γ (PPARγ) , , . In white adipocytes, the transcription factors Krox20 and Klf4 are upstream regulators of C/EBPβ ,  whereas brown fat-specific differentiation requires the interaction of C/EBPβ with the zinc finger-containing protein PRDM16, which leads to adipogenic development through induction of PPARγ and mitochondrial biogenesis through subsequent activation of peroxisome proliferator-activated receptor γ-coactivator 1α (PGC-1α). Whereas genetic inactivation of PPARγ prevents adipocyte development, inactivation of C/EBPβ is still compatible with both white and brown adipose tissue development but prevents normal function of brown fat , .
In a recent study we identified Plac8, also called onzin, as a novel upstream regulator of the brown adipocyte differentiation program. Plac8, a 124 amino acid long protein, shows structural similarity with the product of the fruit weight 2.2 (fw2.2) gene, which controls fruit weight in tomato, through a regulation of cell number. In plants there are many fw2.2-related genes whereas in mammals Plac8 appears to be the unique member of this family . Plac8 contains a cysteine-rich sequence located between amino acids 23–66 (the Plac8 domain). We showed in a recent report that upon induction of brown preadipocyte differentiation Plac8 transiently interacts with C/EBPβ. The Plac8/C/EBPβ complex then binds to tandem C/EBPβ binding sites present on the C/EBPβ gene promoter to induce this gene transcription. Interaction of Plac8 with C/EBPβ requires the initial part of the cysteine-rich region (a.a. 28–38) and Plac8 deletion mutants lacking this sequence can no longer rescue the differentiation of Plac8−/− brown preadipocytes. Plac8−/− mice have abnormal brown adipocytes characterized by a single large lipid droplet and impaired thermogenesis leading to lower body temperature and cold intolerance . Over time, these mice develop obesity for reasons that may be related to defects in thermogenesis and, because Plac8 is also expressed in white adipocyte, to a defect in this tissue homeostasis.
Therefore, here, we investigated the impact of Plac8 inactivation on white adipocyte differentiation in vitro and on white adipose tissue in Plac8−/− mice. We show that Plac8 is required for in vitro adipogenesis through a regulation of C/EBPβ expression and in vivo it is dispensable for white fat depots production but is required to properly control white fat mass.
Material and Methods
Plac8−/− mice on a pure C57Bl/6 background were obtained from Dr Koller's laboratory (University of North Carolina) . C57Bl/6 and Plac8−/− mice were crossed to obtain Plac8+/−, and then Plac8+/− mice were crossed to obtain Plac8+/+,, Plac8+/− and Plac8−/− littermates. Mice were maintained at 24°C on a 12 h/12 h light/dark cycle (7:00–19:00 h), with free access to water and standard chow diet (n° 3436 from Provimi Kliba AG, Kaiseraugst, Switzerland) and were used when 24–29 weeks old when the obesity was established. All animal studies were approved by the Veterinary Office of Canton de Vaud, Switzerland.
Glucose, free fatty acids and triglycerides measurements
Blood samples were obtained from retroorbital bleeding in fed state or after a 16-hour overnight fasting in 24-weeks-old male mice. Analyses were performed using the Roche/Hitachi Robot 902 (Roche Diagnostics) and Roche kits (Roche, Basel, Switzerland).
Histology and morphometry
Visceral and subcutaneous adipose tissues from 29-weeks-old male mice were embedded in paraffin and 5 µm sections were prepared for hematoxylin and eosin staining. Hematoxylin-eosin images from subcutaneous and visceral adipose tissues were used for morphometric analysis using the AxioVision 4.0 software (Zeiss, Oberkochen, Germany). 100 cells were measured using the software per animals.
RNA extraction and real-time PCR
Total RNA was prepared from white adipose tissues from 29-weeks-old male mice or cultured cells using peqGOLD TriFast reagent according to the manufacturer's instructions (Axonlab, Baden, Switzerland). First strand cDNA was synthesized from 0.5 µg of total RNA using random primers (Promega, Mannheim, Germany) and Superscript II RNase H- (Invitrogen, Carlsbad, CA). Real time PCR was performed using Power SYBR Green Master Mix (Applied Biosystem, Foster City, CA, USA). Specific mouse primers for each gene were used and are described in Table S1. All reactions were normalized to cyclophilin levels and performed in triplicate.
Cells protein extraction and Western blot analysis
Cells were lysed using a RIPA buffer containing SDS 0.1% and protease inhibitors (Roche, Basel, Switzerland). Western blot analysis was performed as previously described . 20 mg of total protein were loaded on a 12% SDS-PAGE for each sample. Rabbit anti-Plac8 antibody was obtained from Dr. Koller's laboratory  and used at a dilution of 1/2500, rabbit anti-α-actin (Sigma, A2066, St-Louis, MO) and peroxidase conjugated anti-rabbit IgG (Amersham, NA934V, Glattbrugg, Switzerland) were used as secondary antibodies at a dilution of 1/1000. SuperSignalR West Pico Stable Peroxide solution (Pierce, 1859674, Rockford, IL) was used for chemiluminescent detection.
Generation of retroviral constructs and retroviral transductions
Plac8 cDNA was inserted in pMSCV retroviral vectors (Clontech, Mountain View, CA) with puromycin or hygromycin selection markers. C/EBPβ pMSCV retroviral construct was kindly provided by Dr. Kivanc Birsoy (Massachussets Institute of Technology, MA). Viral constructs were transfected using the calcium-phosphate protocol previously described  into Phoenix packaging cells (Pr. G. Nolan, Standford) along with constructs encoding gag-pol and the VSV-G protein and supernatants were harvested after 48 h in presence of 3 mM of trichostatin A (Sigma, St-Louis, MO) and either used immediately or snap frozen and stored at −80°C for later use. Viral supernatants were added to the cells for 6 hours in the presence of Polybrene (8 mg/ml, Sigma, St-Louis, MO), and then diluted twice with fresh medium. Next day, the viral supernatant was removed and replaced by fresh medium. Each transduction experiment was repeated three times.
MEF preparation and Cell culture
Mouse embryonic fibroblasts were isolated from Plac8+/+, Plac8+/− and Plac8−/− day 14 embryos using the following protocol. Whole embryos was sliced in small pieces and incubated at 37°C for 1 hours in ES trypsin buffer (2.5 mg trypsin, 0.4 mg EDTA, 7 g NaCl, 0.3 mg Na2HP04, 0.24 mg KH2PO4, 0.37 mg KCl, 1 mg dextrose, 3 mg Tris and 1 ml Difco phenol Red, pH 7.6). Then add 4 ml of DMEM (Gibco, Carlsbad, CA) with 10% FBS (Gibco, Carlsbad, CA,) and mixed the digested embryos. Add another 15 ml of medium and incubate the dispersed cells in a T75 flask. After 48 hours, split the cells to two T175 flasks. The primary mouse embryonic fibroblast can be used until passage 8–9. MEF and 3T3-L1 cell line (ATCC, http://www.lgcstandards-atcc.org/) were cultured in DMEM supplemented with FBS at 5% CO2. Cells were allowed to grow to confluence in either 100-mm or 60-mm dishes in DMEM with 10% FBS. Once confluence was reached, cells were exposed to differentiation medium containing dexamethasone (1 mM), insulin (5 mg/ml), isobutylmethylxanthine (0.5 mM). After 2 days cells were maintained in medium containing insulin (5 mg/ml). Medium was changed every other day. Full differentiation was achieved after 7 days.
Oil red O staining
After 7 to 10 days of differentiation, cells were washed once in PBS and fixed with formaldehyde (Formalde-fresh; Fisher, Waltham, MA) for 15 minutes. The staining solution was prepared by dissolving 0.5 g oil-red-O (Sigma, St-Louis, MO) in 100 ml of isopropanol; 60 ml of this solution was mixed with 40 ml of distilled water. After 1 hour at room temperature the staining solution was filtered and added to dishes for 4 hours. The staining solution was then removed and cells were washed twice with distilled water.
The 3 kb C/EPBβ promoter in pGL3 plasmid was a gift from Dr Kivanc Birsoy (Boston, MA). The pMSCV retroviral plasmid for Plac8 was used as expression vector. The 1.3 kb Krox20 promoter was obtained from Addgene (http://www.addgene.org/). 3T3-L1 preadipocytes cell line were transfected at 80% confluence using Lipofectamine™ LTX Reagent (Invitrogen, Carlsbad, CA) as per the manufacturer's protocol. A ß-galactosidase expression vector was co-transfected into cells as a control for transfection efficiency. Luciferase and ß-galactosidase activity were assessed 2 days after differentiation using the Galacto-Star luciferase reporter assay (Roche, Basel, Switzerland) following the manufacturer's instructions. Transfections were performed in triplicate and repeated three times. Statistics were performed using the Student t-test.
shRNAs were constructed using the pSIREN RetroQ vector (Clontech, Mountain View, CA). Two different target sequences for Plac8 were designed by querying the Whitehead siRNA algorithm (http://jura.wi.mit.edu/bioc/siRNAext/) as well as the siRNA designer software from Clontech (http://bioinfo.clontech.com/rnaidesigner/). The sequences chosen for Plac8 were TCGTGACTCAACCTGGATT and ACGGCATTCCTGGATCTAT. Retroviral production, transduction of 3T3-L1 cell line and differentiation protocols were as described above. Oil-red-O staining was performed at day 7. Each experiment was repeated three times.
VAT and SCAT tissues from 29-weeks-old male mice were homogenized with a Polytron in 1.5 ml PBS containing protease inhibitors (Roche, Basel, Switzerland), followed by a centrifugation at 11000 RPM for 5 minutes. The supernatant was placed in another tube for the DNA content assay. DNA content was measured using the Hoechst Method .
Statistical analyses were performed using the Graphpad Prism 4.0 software (Graphpad Software Inc.). Comparisons between groups were performed using the Student t-test.
To evaluate the role of Plac8 in white adipogenesis we first assessed the pattern of Plac8 expression during differentiation of 3T3-L1 adipocytes. Figure 1A shows that upon induction of differentiation, there was a rapid and transient induction of Plac8 expression, which corresponded closely to the pattern of expression of C/EBPβ and Krox20, two transcription factors required early during white fat differentiation. ShRNA-mediated down-expression of Plac8 reduced 3T3-L1 differentiation as determined by Oil Red O (ORO) staining (Figure 1B); this was associated with reduced expression of Plac8 protein and mRNA levels, as well as a reduced expression of C/EBPβ, Klf4, C/EBPδ, Krox20, Pparγ2 and Ap2 (Figure 1C,D). Expression of other adipocyte-specific genes, Ebf1, Gata3, Nur77 and cyclinD1 were, however, not affected by Plac8 knockdown (Figure S1). With shRNA-mediated knockdown of Plac8, addition of rosiglitazone, a potent PPARγ agonist, also failed to restore the full differentiation of 3T3-L1 cells, as shown by ORO staining and gene expression analysis (Figure S2).
A, Time-course (0, 3, and 6 h, 1 to 7 days) of Plac8, C/EBPβ and Krox20 mRNA expression during 3T3-L1 cells differentiation. Three independent experiments are shown. B, Oil red O staining of 3T3-L1 transduced with two different Plac8 (sh1 and sh2 and a control (shLuc) shRNAs at 7 days after induction of differentiation. Upper row: culture dishes; lower row: photomicrographs of the cells (scale bars = 100 µm). C, Western blot analysis of Plac8 protein in shRNA-transduced 3T3-L1 cells at day 0 and 3 and 6 hours after induction of differentiation. Actin served as loading control D, mRNA levels of Plac8 and of the transcriptional regulators C/EBPβ, C/EBPδ, Krox20, Klf4 and PPARγ2 and of the general adipogenic gene aP2 at day 0 and 7 of differentiation. One representative experiment out of three is shown. Values are means ± SD, n = 3.,*p<0.05 vs. shLuc, #p<0.05 vs. shLuc at day 0.
To determine whether overexpression of Plac8 could increase differentiation, 3T3-L1 preadipocytes were transduced with Plac8-expressing retroviruses (Figure 2). This led to increased Plac8 expression and differentiation of 3T3-L1 adipocytes as revealed by ORO staining and by expression of C/EBPβ, C/EBPδ, Krox20, PPARγ2 and aP2 (Figure 2A, B, C).
A, 3T3-L1 cells were transduced with Plac8 or control retroviruses. Oil red O staining was performed at 7 days after induction of differentiation. Upper row: culture dishes; lower row: photomicrographs of the cells (scale bars = 100 µm). B, Western blot analysis of Plac8 in shRNA transduced 3T3-L1 cells at day 0 and 3 and 6 hours after induction of differentiation. Actin served as loading control C, mRNA levels of Plac8 and of the transcriptional regulators C/EBPβ, C/EBPδ, Krox20 and PPARγ2 and of the general adipogenic gene aP2 at days 0 and 7 of differentiation. One representative experiment out of three is shown. Values are means ± SD, n = 3.,*p<0.05 vs. shLuc, #p<0.05 vs. shLuc at day 0.
As another model to assess the requirement for Plac8 to induce adipogenesis, we established embryonic fibroblasts (MEF) from control, Plac8+/− and Plac8−/− mice. Differentiation of wild-type MEF into ORO positive cells was readily achieved with the differentiation cocktail. Differentiation of the heterozygous mutant MEF was less efficient and almost undetectable in the knockout MEF (Figure 3A), as also revealed by measuring expression of aP2, PPARγ2 and adiponectin. We attempted to rescue differentiation of Plac8 knockout MEF by retroviral transduction of Plac8. However, in the absence of Plac8, MEF proliferate extremely slowly, in agreement with a previous report showing that knockdown of Plac8 markedly reduces cell proliferation rate . This decreased proliferation rate prevented retrovirus-mediated gene transduction.
A, Oil red O staining of primary mouse embryonic fibroblasts from Plac8+/+; Plac8+/− and Plac8−/− mice 7 days after induction of differentiation. Upper row: culture dishes; lower row: photomicrographs of the cells (scale bars = 50 µm). B, mRNA expression of aP2, PPARγ2 and adiponectin at day 0 and day 7 after induction of differentiation. One representative experiment out of three is shown. Values are means ± SD. *p<0.05 vs. Plac8+/+ at day 7, #p<0.05 vs. Plac8+/+ at day 0.
To get another independent assessment of the role of Plac8 in white adipogenesis, we transduced NIH 3T3 cells with C/EBPβ, which is known to allow adipocyte differentiation in the presence of rosiglitazone. Figure 4 shows that Plac8 by itself did not induce significant ORO accumulation (Figure 4A) but is an inducer of C/EBPβ (Figure 4B). However, when transduced together with C/EBPβ it led to a marked increase in ORO staining and expression of aP2, resistin, and adiponectin as compared to C/EBPβ transduction alone (Figure 4A,B).
A, NIH-3T3 cells were transduced with Plac8 and C/EBPβ, or control retroviruses and Oil red O staining was performed 7 days after induction of differentiation. Upper row: culture dishes; lower row: photomicrographs of the cells (scale bars = 50 µm). B, mRNA levels of the Plac8, C/EBPβ and aP2 and of the white fat genes adiponectin and resistin at days 0 and 7 after induction of differentiation. One representative experiment out of three is shown. Values are means ± SD, n = 4. *p<0.05 vs. Plac8+/+ at day 7, #p<0.05 vs. Plac8+/+ at day 0, $p<0.05 vs. Plac8−/− at day 7. C, Plac8 transactivates C/EBPβ and Krox20 promoters in 3T3-L1 preadipocytes. Transcriptional activity of a 3 kb C/EBPβ promoter-luciferase reporter construct (black bars) or empty vector (pGL3) (white bars, close to the zero level and not visible) cotransfected into 3T3-L1 preadipocytes with a Plac8 expression or an empty vector. Luciferase activities were determined 48 hours after transfection. Results are means ± SD (n = 3), one representative experiment is shown. *p<0.05 vs. empty vector.
The above data therefore indicated that Plac8 was required for white adipogenesis in 3T3-L1 cells, MEF, and NIH 3T3 cells. They also suggested that Plac8 was an inducer of C/EBPβ expression. This was directly tested by C/EBPβ-promoter reporter assays in transfected 3T3-L1 adipoyctes. As shown in Figure 4C, co-transfection of Plac8 with the C/EBPβ reporter construct markedly increased luciferase activity of the reporter construct.
Mice with genetic inactivation of Plac8 develop late-onset obesity . To assess whether the obesity phenotype was associated with defect in white adipocytes, we first performed histological analysis of visceral and subcutaneous white fat depots. Figure 5A, B, C shows that white adipocytes from both fat depots from heterozygous and homozygous Plac8 knockout mice had increased size. Weight measurements showed increased visceral and subcutaneous fat mass in heterozygous and homozygous knockout mice (Figure 5D). Importantly, however, the total DNA content of these fat depots was lower in the Plac8 knockout mice indicating that even though their mass was greater, the number of cells forming these tissues was smaller (Figure 5E).
Hematoxylin-eosin staining of VAT (A) and SCAT (B) sections of 29-weeks-old Plac8+/+, Plac8+/− and Plac8−/− mice (scale bars = 50 µm). C, Analysis of VAT and SCAT adipocytes size distribution of Plac8+/+, Plac8+/− and Plac8−/− mice. D, VAT and SCAT weight in Plac8+/+, Plac8+/− and Plac8−/− mice. E, Total DNA content in VAT and SCAT of the same mice. Values are means ± SEM (n = 7–13). *p<0.05 vs. Plac8+/+.
Gene expression analysis revealed that this was associated with reduced expression of C/EBPβ, C/EBPα, and PPARγ2 in both VAT and SCAT but no significant reduction of C/EBPδ and aP2 (Figure 6A,B). These data therefore indicated that absence of Plac8 led to reduced total number of white adipocytes but enlargement of the existing ones and reduced expression of critical adipogenic transcription factors. Analysis of lipolytic and lipogenic gene expression showed that, in visceral adipose tissue, the levels of Acc1 and Srebp-1c were normal but those of Fas and Scd-1 were increased in Plac8−/− but not Plac8+/− adipose tissue (Figure 7A). Expression of the lipolytic genes Atgl and Hsl were, however, not different between geneotypyes (Figure 7B). In subcutaneous fat, there was no change in srebp-1c expression but reduced expression of Acc1, Fas and Scd-1 and no change in Atgl and Hsl (Figure 7C,D). Expression of the inflammatory cytokines TNFα and Il-6 was not increased in the adipose tissue of Plac8 knockout mice (not shown).
mRNA levels of the transcriptional regulators C/EBPβ, C/EBPα, PPARγ2, C/EBPδ and of aP2 in VAT (A) and SCAT (B) of 24 weeks-old Plac8+/+, Plac8+/− and Plac8−/− mice. Values are means ± SEM (n = 7–13), *p<0.05 vs. Plac8+/+.
mRNA levels of the lipogenic genes Acc1, SREBP-1c, Fas and SCD-1, and of the lipolytic genes Atgl and Hsl in VAT (A,B) and (C,D) of 24 weeks-old Plac8+/+, Plac8+/− and Plac8−/− mice. Values are means ± SEM (n = 7–13), *p<0.05 vs. Plac8+/+.
As defect in brown fat function and obesity are often associated with abnormal glucose homeostasis, we measured plasma glucose, free fatty acid, and triglyceride concentrations in fed and fasted control and Plac8−/− mice. Figure 8A, B, C show that these parameters were indistinguishable between control and knockout mice.
This study demonstrates that Plac8 is required for in vitro white fat adipogenesis. In vivo, however, Plac8 is dispensable for the formation of white adipocytes but its absence leads to obesity with apparently fewer but greatly enlarged adipocytes. The defect in thermoregulation and increased adiposity are, however, not associated with changes in glucose homeostasis nor in plasma free fatty acid and triglyceride levels.
Plac8 is expressed in both white and brown fat and in both tissues it is enriched in the stromal-vascular fraction containing preadipocytes. General Plac8 inactivation in mice leads to a phenotype of cold intolerance that can be explained by impaired fat oxidation and thermogenesis by brown adipose tissue . The late-onset obesity may, however, result from combined defects in both brown and white fat differentiation and function. Here, our studies aimed to determine the role of Plac8 in white adipogenesis and in white fat in Plac8−/− mice.
In vitro, absence of Plac8 expression prevented differentiation into adipocytes of 3T3-L1 preadipocytes, of NIH 3T3 cells, and of MEF derived from Plac8−/− mice. Kinetics analysis of transcription factor expression upon induction of 3T3-L1 adipocytes differentiation revealed that Plac8 expression peaked at ~3 hours, a kinetics similar to that of Krox20 and C/EBPβ expression. Analysis of Krox20, Klf4, and C/EBPβ expression in 3T3-L1 cells in which Plac8 was knocked down showed that their expression was reduced. In vivo, Plac8−/− visceral and subcutaneous fat tissues showed reduced expression of C/EBPβ, C/EBPα and PPARγ2. These data therefore suggested that Plac8 is an upstream regulator of the adipogenic transcription cascade. This is in agreement with our studies in BAT preadipocytes, which showed that Plac8 is an upstream regulator of C/EBPβ transcription . This was also confirmed by demonstrating that Plac8 activated the transcriptional activity of a C/EBPβ promoter reporter construct expressed in 3T3-L1 adipocytes. Quantitative RT-PCR analysis also showed that absence of Plac8 led to a reduced expression of Klf4 and Krox20, two factors required early for induction of adipogenesis ,  and which acts, at least in part, through induction of C/EBPβ. Thus, Plac8 appears as an upstream regulator of adipogenesis, acting rapidly after induction of differentiation to trigger the adipogenic transcription cascade.
In our present studies differentiation of 3T3-L1 and NIH3T3 cells could be increased by Plac8 transduction, which ensures a stable protein expression for periods of time that are much longer than the transient induction seen upon induction of preadipocyte differentiation. Because Plac8 has been reported to increase the proliferation of certain cell types ,  and that adipogenic differentiation requires growth-arrest, the adipocyte differentiation we observed here may underestimate of the role of Plac8 since it can induce two apparently opposed cellular effects. On the other hand, the adipogenic function of Plac8 depends on its transient interaction with C/EBPβ, an event that immediately follows the induction of differentiation, possibly as a result of posttranslational modifications induced by the differentiation cocktail . So far, there is no information about Plac8 posttranslational modifications, or its interaction with posttranslational modifications of other proteins. This information is required to fully understand how Plac8 contributes to increased adipogenesis.
Plac8 is a relatively small protein consisting of 124 amino acids containing an evolutionarily-conserved cysteine-rich domain that directs interaction with other proteins. Because Plac8 does not have any structural motif usually associated with transcription factors and due to its small size, its function in adipogenesis is probably to regulate the cellular localization, function, or stability of other proteins, such as through its binding to C/EBPβ, which is required for the C/EBPβ-Plac8 complex to bind to the C/EBPβ promoter to induce this gene transcription .
In vivo, Plac8 is not absolutely required for either brown or white fat differentiation since both tissues are present in the Plac8−/− mice. This observation is analogous to that found, for instance with C/EBPβ or Klf15. Suppressed activity of either gene in 3T3-L1 fibroblasts prevents their adipogenic differentiation but knockout of either gene in mice does not prevent appearance of white fat depots , , , . In Plac8−/− mice absence of Plac8 leads to a decreased expression of important adipogenic genes such as C/EBPβ, C/EBPα and PPARγ2 but not of other genes such as C/EBPδ and aP2. This, however, does not prevent augmented fat storage in this tissue. Obesity is usually associated with increase in both adipose cell number and cell size , , . Interestingly, in Plac8−/− mice obesity is not associated with increased cell number but our data rather suggest a decrease in total adipocyte number. This suggests, that even though adipogenesis during development may proceed normally, the recruitment of new adipocytes from preadipocytes during the adult age may be defective even though the fat storage capacity of existing adipocytes is preserved. This fat cell enlargement occurs in the absence of changes in lipolytic gene expression and with an opposite regulation of lipogenic gene expression, which were increased in VAT (fas and scd-1) whereas these genes and acc-1 were decreased in SCAT. The meaning of this opposite regulation is not yet clear.
Decreased BAT activity and increased white fat mass are thought to favor deregulation of glucose homeostasis. However, in the normal chow fed, 29 weeks-old control, Plac+/− Plac8−/− mice studied here fed and fasted glycemia as well as plasma free fatty acids and triglycerides were indistinguishable. This, therefore, suggest that in the conditions studied the defects in thermoregulation and increased white fat mass were not causing major deregulation of glucose homeostasis. We cannot, however, exclude the presence of subtle deregulations in glucose or lipid metabolism, which would require more detailed analysis.
In summary, our data show that Plac8 is required for in vitro adipogenesis and functions upstream of C/EBPβ and possibly Krox20 and Klf4 in triggering adipogenesis. In vivo, Plac8 is dispensable for the production of WAT and BAT. However, because there are fewer white adipocytes in Plac8−/− mice, this suggests that the recruitment of new adipocytes during adult life may be impaired and that the phenotype of the Plac8−/− mice depends on complex interactions between defects in both white and brown adipose tissues.
Plac8 knockdown in 3T3-L1 decreases adipogenesis. mRNA levels of the transcriptional regulators Ebf1, Gata2, Gata3, Nur77 and of Cyclin D1 during differentiation of Plac8 shRNA1 and 2 and control transduced 3T3-L1 cells at day 0 and 7. One representative experiment out of three is shown. Values are means ± SD, n = 3,*p<0.05 vs. shLuc, #p<0.05 vs. shLuc at day 0
Rosiglitazone does not restore the full adipogenic phenotype in shRNA expressing 3T3-L1 cells. A, Oil red O staining of 3T3-L1 transduced with two different shRNA against Plac8 or the control shRNA (shLuc) at 7 days after induction of differentiation in the presence of rosiglitazone in the differentiation cocktail. Upper row: culture dishes; lower row: photomicrographs of the cells (scale bars = 100 µm). B, mRNA levels aP2 and PPARγ2 during at day 0 and 7 of differentiation. One representative experiment out of three is shown. Values are means ± SD, n = 3.,*p<0.05 vs. shLuc, #p<0.05 vs. shLuc at day 0.
We thank Anabela DaCosta and the Mouse Metabolic Facility from the CIG (UNIL) for technical assistance.
Conceived and designed the experiments: MJP BT. Performed the experiments: MJP XB. Analyzed the data: MJP BT. Wrote the paper: MJP BT.
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