An inhibitor of K+ channels modulates human endometrial tumor-initiating cells
© Schickling et al; licensee BioMed Central Ltd. 2011
Received: 29 June 2011
Accepted: 2 August 2011
Published: 2 August 2011
Many potassium ion (K+) channels function as oncogenes to sustain growth of solid tumors, but their role in cancer progression is not well understood. Emerging evidence suggests that the early progenitor cancer cell subpopulation, termed tumor initiating cells (TIC), are critical to cancer progression.
A non-selective antagonist of multiple types of K+ channels, tetraethylammonium (TEA), was found to suppress colony formation in endometrial cancer cells via inhibition of putative TIC. The data also indicated that withdrawal of TEA results in a significant enhancement of tumorigenesis. When the TIC-enriched subpopulation was isolated from the endometrial cancer cells, TEA was also found to inhibit growth in vitro.
These studies suggest that the activity of potassium channels significantly contributes to the progression of endometrial tumors, and the antagonists of potassium channels are candidate anti-cancer drugs to specifically target tumor initiating cells in endometrial cancer therapy.
Potassium (K+) ion channels are important contributors to the malignant phenotype in cancer cells and as such have been shown to drive progression of cancers of the breast, prostate, endometrium and brain [1–8]. Multiple mechanisms exist by which K+ channels exert their oncogenic functions. For example, K+ channels have been shown to modulate cell cycle progression to increase cell proliferation as well as promote cytoskeletal remodeling to enhance invasion and migration [9–21]. Inhibitors of K+ channels thus constitute putative anti-cancer drugs [1, 2, 22–26], though to date none of these antagonists have been explored in a clinical trial setting for any type of cancer.
Novel developments in cancer research demonstrate that tumor initiating cells (TIC, also referred to as cancer stem cells) cause the onset and recurrence of cancers [27–29]. Several biological agents that aim to eradicate TIC are currently in phase I/II clinical trials, but a clinical need remains to identify other pharmacologic approaches to prevent TIC-mediated tumorigenesis.
Interestingly, K+ channels genes have been shown to be amplified in cancers, but the roles of K+ channels in TIC and by extension in cancer progression have not been rigorously addressed. In this manuscript, we present novel observations that an inhibitor of multiple types of K+ channels, tetraethylammonium (TEA), abrogates the tumorigenic abilities of a TIC-enriched subpopulation derived from human endometrial cancer cells and thus may represent a therapeutic strategy for endometrial cancer therapy.
Results and Discussion
Earlier studies have suggested that, in certain cancers, K+ channels accelerate tumor growth; however, their role in the cancer progression remains unclear . Herein, we examined the importance of the integrated activity of multiple K+ channels in the establishment of new endometrial tumors and their putative roles in the onset or recurrence of the disease. Cells used in these studies model two clinically relevant types of endometrial cancers: 1) Ishikawa H cells represent a hormone-dependent type (i.e., ER- and PR-positive); and 2) Hec50co cells are a model of a hormone-independent type (i.e., ER and PR-negative) . K+ channels as diverse as voltage-gated (e.g., HERG) and calcium-sensitive (e.g., IKCa) have been reported to regulate the progression of endometrial cancers [31, 32]. Therefore, we utilized tetraethylammonium (TEA), a broad inhibitor of many types of K+ channels, instead of siRNA-mediated silencing of individual K+ channels to examine the general integrated role of voltage-gated, calcium-sensitive, and ATP-sensitive K+ channels in tumorigenesis.
Since newly arising primary and metastatic tumors are thought to reflect the presence of TIC [28, 29, 33], we hypothesized that the observed potentiation of tumorigenicity is due to activation of TIC in our cell models. Therefore, we isolated TIC-enriched subsets from the Ishikawa H and Hec50co cells to examine whether TEA regulates these sub-populations. Identification of the TIC subpopulation from other cancer cell types is challenging due to their rarity and uncertainties as to TIC-specific markers. It has been suggested that one difference between TIC and other cancer cells is a lower rate of cell division and an elevated activity of the enzyme aldehyde dehydrogenase isoform 1 (ALDH1) [28, 29, 33–35]. We utilized both of these properties to identify and isolate the TIC-enriched subpopulation from Ishikawa H and Hec50co endometrial cancer cells. First, we isolated the cells with high ALDH1 activity, ALDH1 (+), and compared their tumorigenic capacity to those with low ALDH1 activity, ALDH1 (-), using mouse xenograft models. Cells with either high or low ALDH1 activity, as determined by ALDEFLUOR assays, were injected into the flanks of nude mice and tumor growth measured 45-60 days later. Figure 1B shows a tumor in the flank of a mouse where 100,000 ALDH1 positive Hec50co cells have been injected (Figure 1B, ALDH1 (+)). In contrast, no tumor formed in the opposite flank that was injected with 100,000 cells with low ALDH1 activity (Figure 1B, ALDH1 (-)). We thus concluded that a population of TIC is present in our cell models and they can be identified by the high activity of ALDH1 enzyme.
It has been suggested that not only TIC themselves but their early progeny also can demonstrate high ALDH1 activity. As a consequence, ALDH1 positive cells contain two sub-populations: (1) the rapidly proliferating early progenitor cells; and (2) TIC with a stem cell-like low proliferation rate or quiescent TIC. Our subsequent approaches therefore were to differentiate TIC in our cell models on the basis of their low proliferative rate in addition to the high ALDH1 activity. Specifically, we visualized potential TIC using a fluorescent cell membrane marker, PKH26, that is incorporated into the living cells. Retention of PKH26 dye in cell membranes is a function of cell division, whereby the more times cells divide, the less dye each cell retains [33, 36]. For these studies, we used a modified clonogenic assay (endosphere culture, see Methods), and we expected that we could use PKH26 fluorescence intensity to differentiate between the proliferating progenitor cells and the slowly dividing or quiescent TIC in endospheres. Here we present images of live Ishikawa H and Hec50co endospheres. The left panel in Figure 1C is a 3-dimensional reconstruction of an Ishikawa H endosphere (Figure 1C, left panel, nuclei, green) where only a few cells, presumed to be TIC (indicated by the white arrows), show high retention of a PKH26 dye (Figure 1C, left panel, PKH26, red). This endosphere was additionally visualized using a transmitted light (Figure 1C, left panel, DIC, grey) and subsequently all images were merged (Figure 1C, left panel, merge, white arrows point at putative TIC). In Hec50co endospheres, (Figure 1C, right panel, nuclei, green) we observed similar distribution of PKH26 dye (Figure 1C, right panel, PKH26, red) where white arrows indicate putative TIC. The fluorescent and transmitted light (Figure 1C, right panel, DIC, grey) images were merged (Figure 1C, left panel, merge, white arrows designate TIC). We thus concluded that putative TIC are present in our cell models and can be identified by the high activity of ALDH1 enzyme. Importantly, these cells may be the originators of new tumor spheres.
We further extended our hypothesis to examine how sustained exposure to TEA affects formation of new colonies/tumors. Due to the neurotoxicity of TEA, we could not utilize mouse xenograft models to test this hypothesis. We therefore examined growth of cell colonies in soft agar supplemented with 10 μmol/L of TEA instead. As we expected, double positive Ishikawa H and Hec50co cells developed colonies in TEA-free agar (Figure 2C, filled bars). As compared to the untreated counterparts, fewer Ishikawa H colonies grew in TEA-supplemented agar (Figure 2C, Ishikawa H, shaded bar), thus demonstrating that continuous exposure to TEA attenuated the tumorigenic ability of these cells. Remarkably, TEA completely abolished growth of Hec50co colonies (Figure 2C, Hec50co). We thus concluded that TEA abrogated the tumorigenic capacity of Ishikawa H and Hec50co cells, and the TEA withdrawal observed in Figure 1A results in augmentation of tumorigenicity.
These findings are significant for several reasons. First, they validate K+ channels as candidate anti-cancer targets to maintain quiescence of TIC. In particular, cancer patients in remission that have high risk of recurrence may benefit from such therapy to prolong disease-free survival. Importantly, other inhibitors that, similar to TEA, non-selectively antagonize K+ channels are FDA-approved to treat human conditions not related to cancer. These drugs may possess therapeutic benefits of TEA without the associated neurotoxicity . Second, many clinically approved anti-cancer drugs may have off-target TEA-like inhibitory actions towards the variety of K+ channels. Termination of therapy with these drugs may lay the foundation for cancer recurrence by virtue of enhancing the tumorigenicity of surviving TIC . Intriguingly, these responses are analogous in ER-, PR-positive Ishikawa H cells and ER-, PR-negative Hec50co cells, implying a common response in molecularly disparate endometrial cancers . The mechanisms whereby TEA regulates TIC function require further research, but may involve inhibitor-induced depolarization of plasmalemmal and/or mitochondrial membranes and subsequent changes in cell cycle . Also, the contribution of two-pore leak K+ channels, including the K2P family, to TIC function remains undetermined since TEA does not inhibit these channels.
In this study, we demonstrate that TEA, an inhibitor of K+ channels, decreased tumorigenicity of human endometrial cancer cells. Importantly, withdrawal of TEA led to a significant potentiation of tumorigenic ability. Our data suggest that TEA alters tumorigenicity by inhibiting growth of TIC-enriched subpopulations with high activity of ALDH1 and a low basal proliferation rate.
Materials and Methods
Tetraethylammonium chloride (TEA), crystal violet, laminin, Dulbecco's Modified Eagle Medium (DMEM):F12, gentamicin, PKH26 dye and Triton-X 100 were purchased from Sigma (St Louis, MO). ALDEFLUOR assays were from StemCell Technologies (Vancouver, BC, Canada). Agar, Hoechst 33258 and SYTO 16 were from Invitrogen (Carlsbad, CA), FBS and 0.25% trypsin/EDTA from Gibco-BRL (Carlsbad, CA). Low adherence tissue culture flasks were from A. Daigger&Company (Vernon Hills, IL) and glass bottom dishes were from MatTek Corp. (Ashland, MA).
Ishikawa H cells were a generous gift from Dr. Erlio Gurpide (New York University). Hec50co cells were developed in our laboratory from parental Hec50 cells also kindly provided by Dr. Gurpide . Cells were maintained in DMEM:F12 medium supplemented with 20% fetal bovine serum (FBS) and 50 μg/ml gentamicin. Antibiotic-free medium was used for the duration of experiments starting at least 24 h before experimentation.
Cells were seeded at 100,000 cells per well in 6-well cluster plates and incubated with 10-5 mol/L of TEA for 48 h. Subsequently, cells were trypsinized and counted using Countess Automated Cell Counter (Invitrogen, Carlsbad, CA). Viability was determined by the trypan blue exclusion.
ALDH1 activity assays
Aldehyde dehydrogenase isoform 1 (ALDH1) activity was assayed using ALDEFLUOR kit according to the manufacturer's instructions. Briefly, an ALDEFLUOR reagent was added to the cells. An aliquot of these cells was removed and. an ALDEFLUOR inhibitor was added to that to serve as a control for background fluorescence. Cells were incubated at 37°C for 40 min and separated into two sub-populations based on fluorescence intensity (highest ALDH1 activity, ALDH1(+); lowest ALDH1 activity, ALDH1(-)) using a 488 nm laser (FACS ARIA II, Becton Dickinson, Franklin Lakes, NJ).
Athymic NCr-nu/nu mice were purchased from NCI at Frederick (Frederick, MD). Mice were maintained in a sterile environment according to guidelines established by the US Department of Agriculture and the American Association for Accreditation of Laboratory Animal Care (AAALAC). Cells were assesses for viability using Hoechst 33258 dye and mice were injected in one flank with 100,000 ALDH1(+) cells and an equal amount of ALDH1(-) cells in the opposite flank. Tumor growth was monitored for 6-8 weeks. Two mice were used per cell line. All procedures were approved by the Institutional Animal Care and Use Committee at University of Iowa and complied with the standards stated in the Guide for the Care and Use of Laboratory Animals.
Cell membrane staining with the fluorescent dye PKH26 was performed according to the manufacturer's instructions. Briefly, 106 cells were re-suspended in 2 mL of reagent buffer and incubated with 1 μL of PKH26. Subsequently, cells were repeatedly washed, seeded onto the tissue culture flasks and propagated for at least 7 days before experimentation.
Fluorescent cell sorting of PKH26/ALDH1 cells
Cells were stained with the PKH26 dye for 7 days, assayed for ALDH1 activity using ALDEFLUOR reagent, and immediately analyzed by flow cytometry using 488 nm/561 nm lasers of FACS ARIA II. First, we obtained a PKH26(+) population of cells, which was then sorted to obtain ALDH1(+) cells. Cells with the highest levels of both PKH26 and ALDH1 were used in subsequent experiments.
Endosphere cultures and imaging
Ishikawa H cells or Hec50co cells stained with PKH26 dye were seeded onto the low adherence tissue culture flasks in DMEM:F12 medium supplemented with 1% FBS. Floating cell spheres were examined 7-10 day later by confocal microscopy. Aliquots of endospheres were transferred onto 35 mm glass bottom dishes pre-coated with mouse laminin. Live cell nuclei were counter-stained with SYTO16 according to the manufacturer's instructions and individual spheres were imaged as stacks of 0.7-1 μm optical slices using 488 nm/561 nm lasers of a LSM 510 laser confocal microscope (Zeiss, Jena, Germany). Subsequently, optical slices were reconstructed into the three dimensional images using LSM Image Browser (Zeiss, Jena, Germany).
Soft agar assays
Assays were performed in 6-well cluster tissue culture plates pre-coated with 0.5% basal agar in DMEM:F12. Cells were over-laid onto the basal agar at 1000 cells per well in DMEM:F12 supplemented with 0.3% agar and 20% FBS. Additionally, where indicated, 10-5 mol/L TEA was incorporated into the cell suspension. The cell colonies (50 cells or more) were visualized 21 days later using crystal violet solution (crystal violet 0.005% and citric acid 0.1%) and counted.
Data was plotted using SigmaPlot 11.0 software (Systat Software, Inc., San Jose, CA). Statistical significance was determined by one-way analysis of variance (ANOVA) and the post hoc Bonferroni's t-test. A p value <0.05 was considered statistically significant.
This study was supported in part by the Biological Sciences Funding Program of the Office of Vice-President for Research of the University of Iowa; the start up fund of the Department of Obstetrics and Gynecology, Carver College of Medicine of the University of Iowa, NIH NCI RO1-99908 (BMS, KKL and VPK) and NIH RO1-CA133114 (DRS and NAB). We thank Kristina W. Thiel for assistance in manuscript preparation.
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