Introduction
Obesity is defined by the accumulation of excessive adipose tissue that can contribute to physical and psychosocial impairment. The prevalence of obesity in the world, particularly in the USA, has increased over the past four decades, with one third of adults in the USA meeting the criteria for obesity [
1]. As a result, there has been an increase in the incidence of obesity-associated cancers [
2‐
4]. More specifically, recent studies suggest that obesity increases the incidence of breast cancer [
5,
6].
Epidemiological studies investigating the role of obesity in breast cancer suggest that obesity increases the incidence of metastatic breast tumors, results in higher rates of incidence of recurrence, and increases mortality. Haakinson et al. found that obese patients are diagnosed with larger primary tumors and had increased incidence of lymph node metastases [
7]. Furthermore, in postmenopausal breast cancer patients, up to 50 % of deaths have been attributed to obesity [
8]. While the link between obesity and breast cancer has been well-documented from epidemiologic analyses, the molecular mechanisms underlying this correlation are not fully defined.
An analysis of the interplay between breast cancer and obesity provides some insights into the underlying pathophysiology. During breast cancer development and progression, a complex multi-step cascade converts normal breast epithelial cells into malignant cells [
9‐
11]. One of the key steps involves the interaction between the epithelial cells and the stromal microenvironment, which contains adipose stromal/stem cells (ASCs) [
12]. Studies have shown that obesity significantly increases the number of ASCs within the adipose tissue. This ASC hyperplasia has been shown to support both angiogenesis and adipogenesis and to alter the gene expression profile of ASCs such that they enhance cancer growth [
13‐
15]. Recently, our group has demonstrated that ASCs isolated from obese patients with body mass index (BMI) ≥30 (obASCs) enhance the tumorigenicity MCF7 breast cancer cells, and alter their gene expression profile [
13]. Additionally, the data showed that the obASCs expressed significantly higher levels of leptin compared to ASCs isolated from lean patients with BMI ≤25 (lnASCs). However, the overexpression of leptin in obASCs and the impact it has on increasing the aggressiveness of tumor cell biology in vitro and in vivo has not been investigated.
The role of leptin produced by obASCs on breast cancer cells (BCCs) was investigated in this study by inhibiting the expression of leptin using a short hairpin RNA (shRNA) knockdown strategy. The obASCs preferentially increased the proliferation, migration, and invasion of several estrogen receptor positive (ER+) BCC lines, including MCF7, ZR75, and T47D, during direct co-culture. Reducing the levels of leptin in obASCs negated their effects on BCCs. Consistent with phenotypic changes, inhibiting leptin expression in obASCs negated alterations to the gene expression profile of BCC after co-culture. Furthermore, reducing leptin levels in obASCs also resulted in a reduction in tumor volume and fewer metastatic lesions in the lung and liver of SCID/beige mice. These results implicate obASC-derived leptin as a key mechanism that alters BCC growth and supports changes to the biology of BCCs into a more aggressive phenotype. The results here suggest that the inhibition of leptin secreted by obASCs may result in reduced tumor volume and metastasis to distant organs, reducing the burden of obesity-associated breast cancers.
Methods
Human subjects
Human ASCs were obtained from 12 Caucasian women (two groups, six donors per group) undergoing elective liposuction procedures, as previously described [
16]. All protocols were reviewed and approved by the Pennington Biomedical Research Center Institutional Review Board, and all human participants provided written informed consent. Briefly, ASCs were isolated from processed liposuction aspirates from the subcutaneous abdominal adipose tissue of lean or obese patients. Liposuction aspirates were incubated in 0.1 % type I collagenase (Sigma , St. Louis, MO) and 1 % powdered bovine serum albumin (BSA, fraction V; Sigma) dissolved in 100 ml of PBS supplemented with 2 mM calcium chloride. The mixture was placed in a 37 °C shaking water-bath or incubator at 75 rpm for 60 minutes and then centrifuged to remove oil, fat, primary adipocytes, collagenase solution and cellular debris. The resulting cell pellet was re-suspended in stromal medium (SM), which consisted of DMEM/F12 (Hyclone, Logan, UT, USA), 10 % FBS (Hyclone), 1 % antibiotic/antimycotic (Fisher Scientific, Houston, TX, USA), and plated in 175-cm
2 flasks. Fresh SM was added every 2–3 days until cells achieved 80–90 % confluence, at which time cells were harvested with 0.25 % trypsin/1 mM EDTA (GIBCO, Grand Island, NY, USA) and cryopreserved prior to experimental use. The mean BMI for the lnASC group was 22.7 ± 1.9, while the mean BMI for the obASCs was 32.7 ± 3.7. The mean age of the subjects for each group of donors was as follows: lnASCs (38.8 ± 7.0 years) and obASCs (42.5 ± 8.9 years). There was no statistically significant difference in age between the donor groups.
Cell culture
ASCs
Frozen vials of ASCs were thawed and cultured on 150-cm
2 culture dishes (Nunc, Rochester, NY, USA) in 25 ml of complete culture medium (CCM) and incubated at 37 °C with 5 % humidified CO
2. After 24 hours, viable cells were harvested with 0.25 % trypsin/1 mM EDTA and re-plated at 100–200 cells/cm
2 in CCM, which consisted of α-Minimal Essential Medium (αMEM; GIBCO), 20 % FBS (Atlanta Biologicals, Lawrenceville, GA, USA), 100 units per ml penicillin/100 μg/ml streptomycin (P/S; GIBCO), and 2 mM L-glutamine (GIBCO). Medium was changed every 2–3 days. For all experiments, sub-confluent cells (≤70 % confluent) between passages 2–6 were used. Characterization of stem cells has previously been performed and published [
13].
Breast cancer cell (BCC) lines
MCF7 (HTB-22), ZR75 (CRL-1500), and T47D (HTB-133) cells were obtained directly from American Type Culture Collection (ATCC; Manassas, VA, USA) and used within 6 months of resuscitation. Cell line authentication was conducted by ATCC via short tandem repeat profiling. Cells were cultured in DMEM (GIBCO), supplemented with 10 % FBS (Atlanta Biologicals) and P/S. Cells were grown at 37 °C with 5 % humidified CO2, fed every 2–3 days, and split 1:4 to 1:6 when the cells reached 90 % confluence.
Synthesis of green fluorescent protein positive (GFP+) BCCs
To produce lentivirus, 293T cells were transfected through a modified calcium chloride transfection protocol when cells reached 70−75 % confluence. For each transfection, 10 μg of packaging plasmid, enveloping encoding plasmid, and transfer plasmid containing GFP and neomycin resistance or dsRed and neomycin resistance were used. After 48 hours, medium was harvested and used to transduce cancer cells. To transduce ASCs, conditioned medium containing virus with dsRed and neomycin resistance was added to ASCs at 70 % confluence. MCF7, ZR75, T47D, and ASCs were selected with 500 μg/ml of Geneticin (Invitrogen; Carlsbad, CA, USA) for 2 weeks and GFP expression or dsRed expression was verified with flow cytometry. All cancer cells and ASCs used for experimentation expressed GFP or dsRed unless otherwise specified.
ASCs pooled from six donors per group, were plated on a 150-cm2 cell culture dish at 100 cells/cm2. After overnight culture, medium was replaced with serum-free αMEM. After 7 days, conditioned media (CM) were collected and filtered to remove cellular debris. The total number of ASCs was also counted to verify equal number of cells after 7 days. ASC CM from lnASCs and obASCs was plated on top of BCCs set up in triplicates. After 7 days, the total number of MCF7 cells was counted. Where indicated, CM was collected from control shRNA lnASCs, leptin shRNA lnASCs, control shRNA obASCs, and leptin shRNA obASCs.
Stable transfection of shRNA
shRNA constructs targeting leptin and an shRNA construct targeting a non-human gene serving as a negative control were purchased from SA Biosciences (Frederick, MD, USA). The GFP sequence in the shRNA construct was removed and replaced with dsRed and neomycin resistance, producing a dsRed, neomycin-resistant leptin shRNA construct and a dsRed, neomycin-resistant negative control shRNA construct. The lnASCs (n = 6 donors) and obASCs (n = 6 donors) were transfected with a dsRed, neomycin-resistant leptin shRNA construct or a dsRed, neomycin-resistant negative control shRNA construct using the Neon Transfection System (Invitrogen), using 1400 V for the pulse voltage, 10 ms for the pulse width, and three pulses. Cells were allowed to recover, expanded, underwent antibiotic selection for 2 weeks, and sorted by flow cytometry to verify dsRed expression. Four groups of cells (n = 6 donors/group) were produced: control shRNA lnASCs, leptin shRNA lnASCs, control shRNA obASCs, and leptin shRNA obASCs.
Alamar blue cell proliferation assay
Alamar blue cell proliferation assay was conducted according to manufacturer’s instructions. Briefly, 100 cells from each donor (lnASCs, control shRNA lnASCs, leptin shRNA lnASCs, obASCs, control shRNA obASCs, or leptin shRNA obASCs) were plated in a 96-well plate in triplicates. After cells had adhered overnight, the medium was removed, the wells were washed three times in PBS, and the cells were incubated in 10 % Alamar Blue reagent (Invitrogen). After 18 hours, the fluorescence intensity was measured at an excitation wavelength of 540 nm and an emission wavelength of 580 nm using a fluorescence plate reader. Cells were assessed on days 1, 3, and 7.
RNA isolation followed by reverse transcriptase polymerase chain reaction (qRT-PCR)
Subconfluent cultures of control shRNA lnASCs (n = 6 donors), leptin shRNA lnASCs (n = 6 donors), control shRNA obASCs (n = 6 donors), and leptin shRNA obASCs (n = 6 donors) were analyzed. RNA was extracted from ASCs using TRIzol reagent (Invitrogen), purified with RNeasy columns (Qiagen, Valencia, CA, USA), and digested with DNase I (Invitrogen). A total of 1 μg of cellular RNA was used for cDNA synthesis with SuperScript VILO cDNA synthesis kit (Invitrogen). Quantitative real-time PCR was performed using the EXPRESS SYBR GreenER qPCR SuperMix Kit (Invitrogen) according to the manufacturer’s instructions. The following primer set sequence for leptin (forward 5′-gaagaccacatccacacacg-3′, reverse 5′-agctcagccagacccatcta-3′) and β-actin (forward 5′-caccttctacaatgagctgc-3′ and reverse 5′-tcttctcgatgctcgacgga-3′) were used. At the completion of the reaction, ΔΔ cycle threshold (ΔΔ Ct) was calculated to quantify mRNA expression.
Characterization of ASCs
ASCs were characterized as previously described [
17]. Briefly, ASCs were induced to undergo osteogenic or adipogenic differentiation. For osteogenic differentiation, ASCs were cultured in 6-well plates in CCM until 70 % confluent and medium was replaced with fresh medium containing osteogenic supplements, consisting of 50 μM ascorbate 2-phosphate (Sigma), 10 mM β-glycerol phosphate (Sigma), and 10 nM dexamethasone. After 3 weeks, cells were fixed in 10 % formalin for 1 hour at 4 °C and stained for 10 minutes with 40 mM Alizarin Red (pH 4.1; Sigma) to visualize calcium deposition in the extracellular matrix. Images were acquired at × 4 magnification using the Nikon Eclipse TE200 (Melville, NY, USA) with the Nikon Digital Camera DXM1200F and the Nikon ACT-1 software version 2.7. For adipogenic differentiation, ASCs were cultured in 6-well plates in CCM until 70 % confluent, and medium was replaced with fresh medium containing adipogenic supplements consisting of 0.5 μM dexamethasone (Sigma), 0.5 mM isobutylmethylxanthine (Sigma), and 50 μM indomethacin (Sigma). After three weeks, cells were fixed in 10 % formalin for 1 hour at 4 °C, stained for 10–15 minutes at room temperature with Oil Red O (Sigma) to detect neutral lipid vacuoles, and images were acquired at × 10 magnification.
To determine the ability to form colony-forming units (CFU), ASCs were plated at a density of 100 cells on a 10-cm2 plate in CCM and incubated for 14 days. Plates were rinsed three times with PBS, and 10 ml of 3 % crystal violet (Sigma) was added for 30 minutes at room temperature. Plates were washed three times with PBS and once with tap water.
Analysis by flow cytometry of the cell surface marker profile was conducted by harvesting ASCs with 0.25 % trypsin/1 mM EDTA for 3–4 minutes at 37 °C. A total of 3 × 105 cells were concentrated by centrifugation at 500 × g for 5 minutes, suspended in 50 μl PBS and labeled with the primary antibodies. The following primary antibodies were used: anti-CD45-PeCy7, anti-CD11b-PeCy5, anti-CD166-PE, anti-CD105-PE, anti-CD90-PeCy5, anti-CD34-PE, isotype-control fluorescein isothiocyanate (FITC) human IgG1 and isotype-control PE human IgG2a were purchased from Beckman Coulter (Indianapolis, IN, USA). Anti-CD44-APC was purchased from BD Biosciences (Franklin Lakes, NJ, USA). The samples were incubated for 30 minutes at room temperature, washed with PBS, and analyzed with the Galios Flow Cytometer (Beckman Coulter, Brea, CA, USA), running Kaluza software (Beckman Coulter). To assay cells by forward and side scatter of light, the FACScan was standardized with microbeads (Dynosphere uniform microspheres, Bangs Laboratories Inc., Thermo Scientific, Waltham, MA, USA). At least 10,000 events were analyzed and compared with isotype controls.
BCC and ASC co-culture
BCCs were co-cultured with lnASCs (n = 6 donors) or obASCs (n = 6 donors) at 200 cells/cm2 in a 1:1 ratio in DMEM supplemented with 10 % FBS (Atlanta Biologicals) and P/S. After 7 days, cells were harvested, washed, and analyzed by flow cytometry. The percentage of GFP+ cells (BCCs) was determined using the Galios Flow Cytometer, running Kaluza software, and calculated based on the total number of cells. Where indicated, control shRNA lnASCs (n = 6 donors), leptin shRNA lnASCs (n = 6 donors), control shRNA obASCs (n = 6 donors), and leptin shRNA obASCs (n = 6 donors) were co-cultured with MCF7, ZR75, or T47D for 7 days. The percentage of GFP+ cells (BCCs) was determined with the Galios Flow Cytometer, running Kaluza software, and calculated based on the total number of cells. For RNA isolation, BCCs were sorted after co-culture with the Becton-Dickinson FACSVantage SE Cell Sorter with the DiVa option (BD, Franklin Lakes, NJ, USA) and analyzed with the DiVa software v5.02 (BD).
Transwell migration and invasion assays
Migration assays were performed in transwell inserts with 8-μm-pore membrane filters, while invasion assays were performed with 8-μm transwell inserts pre-coated with a growth factor-reduced Matrigel layer to mimic basement membranes (BD Biosciences). BCC cells were cultured alone or co-cultured with control lnASCs, leptin shRNA lnASCs, control obASCs, or leptin shRNA obASCs for 7 days in a 1:1 ratio. BCCs were purified with FACS, and 1.25 × 104 BCCs suspended in 50 μl were added to the apical chamber. A total of 200 μl of chemoattractant (10 % FBS; Atlanta Biologicals) was added to the basal chamber and incubated for 4 hours or 24 hours for migration or invasion, respectively. After the allotted time, the lower side of the transwell insert was carefully washed with cold PBS and non-migrating or non-invading cells remaining on the top chamber were removed with a cotton tip applicator. Migrating and invading cells were stained with Calcein-AM (2 μg/ml; Invitrogen) and measured on a fluorescent plate reader (FLUOstar optima, BMG Labtech Inc., Durham, NC, USA). Data were normalized to the respective BCCs without previous exposure to ASCs.
RNA isolation followed by custom RT2 Profiler™ PCR arrays
To assess cells with the PCR array, total cellular RNA was extracted using RNeasy Mini Kit from FACS-purified BCCs cultured alone or after co-culture with a pool of control shRNA lnASCs, leptin shRNA lnASCs, control shRNA obASCs, or leptin shRNA obASCs, with six donors per group (Qiagen). RNA was treated with DNase I (Qiagen) according to manufacturer’s instructions: 1 μg of RNA was converted to cDNA with the RT2 First Strand Kit (SA Biosciences) according to the manufacturer’s protocol. Where indicated, total cellular RNA was extracted from tumors using RNeasy Mini Kit, treated with DNase I, and converted to cDNA with the RT2 First Strand Kit according to the manufacturer’s instructions. Gene expression profiling was performed using a Custom Breast Cancer RT2 Profiler PCR Array (SA Biosciences) and RT2 qPCR Master Mix (SA Biosciences). The Custom Breast Cancer RT2 Profiler PCR Array was manufactured to detect the expression of the following genes: SERPINE1, IGFBP3, GSTP1, MMP-2, SNAI2, IL-6, PGR, TWIST1, PTGS2, SFRP1, THBS1, CDKN2A, PLAU, CSF1, and ACTB. PCR amplification was performed in a Bio-Rad CFX96 Real-Time System (Hercules, CA, USA). The reaction conditions were as follows: 95 °C for 10 minutes, 40 cycles of 95 °C for 15 sec and 60 °C for 1 minute, followed by a dissociation curve. At the completion of the reaction, Ct values were determined, and ΔΔ Ct and fold change were determined using the RT2 Profiler PCR Array Data Analysis web portal (SA Biosciences). Genes with mRNA levels increased or decreased more than two-fold were considered significantly differentially expressed (P <0.05).
In vivo tumorigenicity assay
SCID/beige (CB17.Cg-PrkdcscidLystbg-J/Crl) immunocompromised female ovariectomized mice (5 weeks old) were obtained from Charles River Laboratories (Wilmington, MA, USA). To assess whether leptin impacts tumorigenicity, mice were divided into three groups (n = 5 mice/group): MCF7 cells only, MCF7 cells plus control shRNA obASCs (n = 6 donors), and MCF7 plus leptin shRNA obASCs (n = 6 donors). Estradiol pellets (0.72 mg, 60-day release, Innovative Research of America, Sarasota, FL, USA) were implanted subcutaneously in the lateral area of the neck. Cell implants were prepared with MCF7 cells (106) alone or MCF7 cells (106) in combination with ASCs (106) suspended in a total volume of 150 μl (one part sterile PBS and two parts reduced growth factor Matrigel (BD Biosciences). Cells were injected subcutaneously into the fifth mammary fat pad on both sides. All procedures in animals were carried out under anesthesia using a mixture of isoflurane and oxygen delivered continuously by mask. After 36 days, animals were euthanized by cervical dislocation after exposure to CO2. Organs were removed, weighed, digitally imaged, and fixed in 10 % neutral buffered formalin. Where indicated, additional mice were divided into three groups (n = 5 mice/group): MCF7 only, MCF7 plus lnASCs, and MCF7 plus obASCs to assess for potential metastasis by lnASCs or obASCs. Lungs and livers were also harvested and fixed in 10 % neutral buffered formalin for histological analyses.
All procedures involving animals were conducted in compliance with State and Federal law, standards of the US Department of Health and Human Services, and guidelines established by Tulane University Institutional Animal Care and Use Committee (IACUC). All animal protocols were approved by the Tulane University IACUC.
Flow cytometry
Flow cytometry was conducted on the tumors to assess for GFP expressing MCF7 cells and dsRed expressing ASCs. Tumors were dissociated with collagenase/hyaluronidase (Stem Cell Technologies, Vancouver, BC, Canada) for 16 hours at 37 °C. After enzymatic dissociation, the reaction was neutralized with pre-warmed medium consisting of 10 % FBS (Atlanta Biologicals). Cells were centrifuged at 350 × g for 10 minutes, counted, and resuspended in PBS. The samples were then analyzed with the Galios Flow Cytometer running Kaluza software.
Immunohistochemistry
Formalin-fixed, paraffin-embedded (FFPE) tumor, lung, and liver sections were de-paraffinized, rehydrated in Sub-X (Leica, Buffalo Grove, IL, USA) and graded solutions of ethanol, and stained with hematoxylin and eosin. FFPE tumor sections were de-paraffinized, rehydrated in Sub-X and graded solutions of ethanol, quenched with 0.3 % H2O2 (Sigma), rinsed with Tris-NaCl-Tween buffer (TNT), which consisted of 0.1 M Tris-HCl (pH 7.5; Sigma), 0.15M NaCl (Sigma), and 0.05 % Tween-20 (Invitrogen). Tumor sections were then blocked with 1 % BSA, and stained with primary antibodies obtained from Abcam against GFP, dsRed, SERPINE1, or matrix metalloproteinase-2 (MMP-2) overnight at 4 °C. Each tumor section was subsequently washed in TNT buffer. Tissue sections were incubated with appropriate horseradish peroxidase (HRP)-conjugated secondary antibody (Abcam) for 1 hour at room temperature, and washed with TNT buffer. For colorimetric staining, slides were then incubated in 3,3′-Diaminobenzidine (DAB; Vector Laboratories), washed with TNT, counterstained with hematoxylin (Thermo Scientific), and rinsed with deionized water. Slides were dehydrated in graded solutions of ethanol, followed by SubX in the final step, and sealed with Permount Mounting Medium (Sigma). After staining, images were acquired at × 10 and × 40 magnification with the ScanScope CS2 (Aperio, Vista, CA, USA).
Protein isolation and western blot
Protein lysates were isolated with radioimmunoprecipitation assay (RIPA) buffer (Pierce; Thermo Scientific) from primary tumors formed with MCF7 cells, MCF7 cells mixed with control shRNA obASCs, or MCF7 cells mixed with leptin shRNA obASCs. Tumors were homogenized in RIPA buffer for 5 minutes, and the cell lysate was clarified by centrifugation at 15,000 × g for 15 minutes. Protein concentration was determined by the BCA Protein Assay (Pierce). Lysate (20 μg) was resolved on 4−12 % SDS-polyacrylamide gels and transferred to nitrocellulose membranes (Invitrogen). Blots were blocked with blØk Noise Canceling Reagents (Millipore Billerica, MA, USA). Blots were then incubated with anti-leptin antibody (R&D Systems; Minneapolis, MN, USA) overnight at 4 °C and washed with PBS with Tween 20 three times before being incubated with species-specific IgG conjugated to HRP for 1 hour at room temperature. Antigen-antibody complexes were visualized after incubation in chemiluminescence reagent (Invitrogen). Blots were imaged on an ImageQuant LAS 4000 (GE Healthcare Life Sciences; Piscataway, NJ, USA) and quantitative analysis of western blots was performed with densitometry.
Metastatic lesions were quantified by determining the area occupied by the lesion divided by the total area of the tissue section. The percentage the tissue occupied by metastatic cells in the liver and lung were averaged together for each mouse (n = 5 mice/group) and represented as the metastatic index.
Statistical analysis
All values are presented as means ± standard error of the mean (SEM). The statistical differences among three or more groups were determined by analysis of variance (ANOVA), followed by post-hoc Tukey multiple comparison tests versus the respective control group. Statistical significance was set at P <0.05. Analysis was performed using Prism (Graphpad Software, San Diego, CA, USA).
Discussion
The incidence of obesity has been steadily increasing over the past few decades. Obese and overweight individuals now account for more than two thirds of the adult population in the USA [
18]. Much co-morbidity is associated with obesity, and a clear epidemiological association between obesity and the prevalence of numerous cancers has been established; one being breast cancer [
19]. While the relative risk amongst studies varies from 1.5 to 2.5, there is consensus that there is an increased relative risk of breast cancer development in women with BMI >30 [
20‐
22].
Recent studies investigating the role of adipose tissue on breast cancer, in particular the excessive accumulation of adipose tissue in obesity, implicate ASCs as a significant factor contributing to disease development [
23]. ASCs are stromal/stem progenitor cells of mesenchymal origin and have been shown to travel through the blood to distant tumor sites where they differentiate into vascular pericytes or secrete growth factors that support the tumor microenvironment [
24,
25]. Additional studies suggest that ASCs originating from remote fat depots have the potential to traffic to the tumor and promote tumor progression through the secretion of proteases and pro-angiogenic factors [
15,
26]. In the present study, the impact of obASCs on several BCC lines was investigated. The data presented here indicate that obASCs enhance the proliferation of ER
+ BCCs and the preferential impact of obASC on ER
+ BCC lines suggest that ER
+ BCCs are able to respond to factors produced by the obASCs, which are not produced by lnASCs. Furthermore, the data suggests that TNBC may not express receptors or that their signaling pathways do not respond to the factors produced by obASCs.
Previously, ASCs have been shown to be a source of the leptin in the adipose tissue, and this leptin produced by the ASCs has been shown to stimulate BCC proliferation [
13]. Leptin, a growth factor produced within adipose tissue, primarily functions to maintain energy balance. It also plays an important role in cell growth and differentiation under normal physiological conditions [
27]. Previous studies have also indicated that a leptin-leptin receptor signaling axis may crosstalk with the ER and enhance tumorigenesis and metastasis [
28‐
31]. These findings are consistent with our current report of obASCs and their preferential role in increasing ER
+ BCCs but not ER
− BCCs.
Obesity has been shown to result in hyperleptinemia [
32]. Hyperleptinemia leads to an increase in breast cancer cell proliferation, migration, and invasion, which gives rise to more aggressive and metastatic tumor cells [
33‐
41]. Several laboratories have confirmed that exogenously delivered leptin increases BCC proliferation at different concentrations (100–1,600 ng/ml) [
33‐
40]. Previously, studies have shown that the mechanism by which leptin promotes the survival of cancer cells is through the activation of multiple signaling pathways, such as those involving mitogen-activated protein kinase (MAPK), Janus kinase 2-signal transducer and activator of transcription 3 (JAK2-STAT3) and phosphatidylinositol 3-kinase-protein kinase B (PI3K-AKT) [
42,
43]. However, additional studies are necessary to determine the sources of leptin in the adipose tissue and whether leptin secreted by the obASCs utilizes similar signal transduction pathways to promote the survival of cancer cells.
The mechanism by which obASC-derived leptin promotes alterations to the biology of BCCs was investigated by inhibiting leptin expression by stably transfecting lnASCs and obASCs with a leptin shRNA construct. The data suggest that obASC-derived leptin enhances several central processes such as proliferation and metastasis of cancer cells that ultimately enhance the aggressiveness of breast cancer cells. However, the precise mechanism by which obASC-derived leptin enhances proliferation remains to be determined. Our assessment of several key proliferative factors demonstrated increased expression of CDKN2A and SFRP1 in MCF7 and ZR75 cells following co-culture with obASCs. Inhibiting leptin expression negated the increased expression of CDKN2A and SFRP1 in MCF7 and ZR75 cells even after co-culture, suggesting that the expression of these two genes are leptin-mediated; however, these results did not translate into the T47D cells, which indicate obASC is not signaling through CDKN2A and SFRP1 to increase the proliferation of T47D cells. Therefore, additional analysis utilizing RNA-sequencing or other global approaches to assess gene expression may be warranted in order to assess the broader impact of obASCs and obASC-derived leptin on the proliferation of all ER+ BCCs.
With respect to migration and invasion, obASCs enhanced migration and invasion of BCCs. However, inhibition of leptin only reduced the invasive potential of BCCs. These results suggest that while other factors secreted by obASCs enhance BCC migration, leptin plays an important role in BCC invasion. Studies have shown that migration is largely dependent on integrins and adhesion molecules, while invasion is dependent on the expression of proteases [
44,
45]. Therefore, obASC-secreted leptin likely regulates the expression of proteases.
With respect to metastasis, leptin appears to signal primarily through SERPINE1 and MMP-2 [
46,
47]. SERPINE1, a serine protease inhibitor, limits the activity of matrix metalloproteases in the extracellular matrix microenvironment [
48]. Paradoxically, SERPINE1 is also involved in other molecular interactions, including binding to the extracellular matrix protein vitronectin and endocytosis receptors of the low-density lipoprotein receptor (LRP) family. Binding of SERPINE1 to vitronectin results in detachment of the tumor cell from the extracellular matrix (ECM), leading to enhanced mobility of the cells [
49]. Likewise, MMP-2 expression correlates with increased metastasis and poorer clinical prognosis [
50,
51]. Furthermore, the cells expressing MMP-2 are also important and indicative of the aggressiveness of the breast cancer [
52]. Elevated expression of MMP-2 in cancer cells has been found to be associated with smaller tumors, while expression of MMP-2 by stromal cells has been associated with increased aggressiveness [
52]. Furthermore, expression of IL-6 was similarly upregulated in BCCs following co-culture with obASCs. However, tumors formed with a mixture of leptin shRNA obASCs and BCCs did not demonstrate similar reduction in IL-6, which suggests that other cells within the tumor microenvironment may be contributing to the increase in IL-6. In particular, studies have shown that immune cells express high levels of IL-6 during the cancer progression [
53,
54]. Nevertheless, the elevated expression of SERPINE1 and MMP-2 correlated with the increased incidence of metastatic lesions in the lung and liver of mice injected with a mixture of obASCs and cancer cells, compared to mice that received cancer cells alone or cancer cells mixed with lnASCs. Furthermore, the expression of SERPINE1 and MMP-2 was reduced in tumors formed with cancer cells and leptin shRNA obASCs, relative to tumors formed with cancer cells and control shRNA obASCs. These results suggest that leptin affects the overexpression of these key metastatic factors within the tumor.
Competing interests
JMG is a co-owner, co-founder and Chief Scientific Officer of LaCell LLC, a biotechnology company focusing on the use of stromal/stem cells for regenerative medicine and research. The other authors declare that they have no competing interests.
Authors’ contributions
ALS took part in the conception and design of the study, the collection and assembly of the data, data analysis and interpretation, statistical analysis, and manuscript writing. JFO, BAB, DTP, HAT, CL, and SZ assisted in the in vitro data collection, assembly of data, and drafting the manuscript. LVR, ACB, and MFD performed the in vivo data collection, histological analyses of in vivo samples, and assisted in drafting the manuscript. JMG, MEB, and BAB took part in the conception and design of the study, data interpretation, manuscript writing, and financial support. All authors approved the final manuscript.