Circadian clocks control cell cycle factors, and circadian disruption promotes cancer. To address whether enhancing circadian rhythmicity in tumor cells affects cell cycle progression and reduces proliferation, we compared growth and cell cycle events of B16 melanoma cells and tumors with either a functional or dysfunctional clock.
We found that clock genes were suppressed in B16 cells and tumors, but treatments inducing circadian rhythmicity, such as dexamethasone, forskolin and heat shock, triggered rhythmic clock and cell cycle gene expression, which resulted in fewer cells in S phase and more in G1 phase. Accordingly, B16 proliferation in vitro and tumor growth in vivo was slowed down. Similar effects were observed in human colon carcinoma HCT-116 cells. Notably, the effects of dexamethasone were not due to an increase in apoptosis nor to an enhancement of immune cell recruitment to the tumor. Knocking down the essential clock gene Bmal1 in B16 tumors prevented the effects of dexamethasone on tumor growth and cell cycle events.
Here we demonstrated that the effects of dexamethasone on cell cycle and tumor growth are mediated by the tumor-intrinsic circadian clock. Thus, our work reveals that enhancing circadian clock function might represent a novel strategy to control cancer progression.
Tumor cells are characterized by uncontrolled cell proliferation resulting in abnormal and accelerated tissue growth. In contrast, “healthy” cells often proliferate with a division rate of ~24 h . This is due to the direct control of cell cycle checkpoints by the intracellular circadian clock machinery .
Circadian clocks operate in most tissues at the single-cell level . At the molecular level, these clocks are based on clock genes, which participate in auto-regulatory feedback loops. In the core loop, the transcription factors CLOCK and BMAL1 activate the expression of Per and Cry genes, whose protein products negatively feed back on their own expression . Several additional feedback loops contribute to this canonical mechanism, including one involving the nuclear receptor NR1D1. Moreover, in any given cell type, 5–20% of the transcriptome is under circadian control . This is the basis for circadian control of major physiological processes, including immune functions and, most importantly for this investigation, cell proliferation [2, 6].
Misalignment between the external and internal time and circadian disruption, such as during shift work, has been associated with an increased cancer risk [7–10] and promotes tumor growth [11–13]. Moreover, circadian clock alteration due to mutations of single clock genes, such as Per2 or Bmal1, accelerates tumor growth [14, 15] or the whole carcinogenesis process [16–18]. This is putatively due to an increase in proliferation rate upon circadian rhythm disruption, because tumor suppressor and key cell cycle genes are under clock control [2, 3] in the context of a bidirectional clock–cell cycle coupling [19, 20]. In support of the connection between rhythm disruption and oncogenesis, deregulated circadian rhythms appear to be a common feature of cancer cell lines [14, 21] and advanced-stage tumors . Moreover, in mouse models of tumorigenesis, the outcome of the disease correlates with the level of improvement of circadian rhythmicity [22, 23]. Intriguingly, cancer prognosis and survival has been associated with the level of circadian disruption in patient tumor tissues [24, 25]. Although a previous study suggested a role for the circadian clock within cancer cells in tumor growth , direct evidence has been missing. Here, we show that improving circadian rhythms in the tumor slows down cell cycle progression and strongly reduces proliferation and tumor growth.
The general objective of the study was to investigate the role of the tumor cell-intrinsic circadian clock in relation to cell proliferation in culture and tumor growth in mice. For this purpose, we activated the circadian clock in B16 melanoma cells and subcutaneous (s.c.) B16 tumors and compared cell cycle gene expression, cell cycle phase distribution and tumor growth after repeated dexamethasone (DEX) or phosphate-buffered saline (PBS) treatment under controlled laboratory experimental conditions. We repeated those experiments using Control or Bmal1 short hairpin RNA (shRNA)-transfected B16 tumors as a model with an inducible or non-inducible circadian clock. In the in vitro experiments, other clock-enhancing treatments (forskolin, heat shock) were also used. Further, we used NOD-scid IL2Rgammanull (NSG) mice to exclude the possible role of DEX on immune infiltration in the tumors. HCT-116 cells and tumors were used to extend the data obtained from B16 melanoma cells to another cancer cell line, from human origin. In all animal experiments, mice were killed after 7–13 days of treatment and during the second day in constant darkness at the indicated circadian hours. The sample size could change during an experiment when the tumor size reached the previously defined clinical endpoint of individual mice and animals had to be killed. The sample size of all biological replicates per time point is indicated in each figure legend or the related tables (in Additional file 1), and mice were randomized between all groups. The study was not performed double-blinded: the experimenter was not blind to the identity of the animal in the different groups, because the treatment of each animal had to be performed according to the specific group. None of the animals was excluded from the analysis or the statistics.
Cell culture and bioluminescence recordings
The B16 and HCT-116 cell lines, developed from murine skin and human colonic carcinoma [26, 27], were obtained from Drs Hua Gu (Institut de Recherche Clinique de Montréal, Montréal, QC, Canada) and Dindial Ramotar (University of Montréal, Montréal, QC, Canada), respectively, and cultured using standard conditions. Stable transfections with luciferase reporters were done according to standard procedures. More details can be found in the Additional file 2. All cell lines tested negative for Mycoplasma. B16 cells express the glucocorticoid receptor  and HSF1 , the latter being relevant for circadian synchronization by heat shock . HCT-116 cells seem not to express functional glucocorticoid receptors . However, steroids such as glucocorticoids can act through glucocorticoid receptor-independent pathways  and the synchronization of circadian rhythms in HCT-116 cells can be achieved by DEX treatment .
For whole-culture imaging, B16 cells or 200 μm slices of tumors from B16 cells with luciferase reporters were cultured in sealed dishes and recorded in a LumiCycle luminometer (Actimetrics Inc., Wilmette, IL, USA). Overall brightness was calculated by averaging values from 12 h after the start of recording to the end of recording. For single-cell imaging, B16 cells or B16 tumor slices were cultured under a microscope inside an incubator, and recorded using a charge-coupled device camera (Ikon-M 934BV Series, Andor Technology, Belfast, UK). Images were collected at intervals of 30 min, with 29 min exposure duration. Data were smoothed by a running minimum algorithm, and bioluminescence intensity was measured within a region of interest with a constant size, but defined manually for each moving cell. Detailed conditions and data analysis can be found in Additional file 2.
Bmal1 shRNA or Scrambled shRNA Lentiviral Particles (Creative Biogene, Shirley, NY, USA) consist of a pool of three constructs encoding 19–25 nt long target-specific shRNA, or shRNA with the same sequence composition, but scrambled. We ensured that the sequences of Bmal1 shRNAs were absent in the mouse genome. B16 cells were grown in 12-well plates until 50% confluency. The medium was replaced with antibiotic-free Opti-MEM medium with 5 μg/mL Polybrene (Sigma-Aldrich, St. Louis, MO, USA). Cells were infected by the addition of 1 × 105 infectious units of virus. After 24 h, the medium was replaced with regular growth medium. Stable clones expressing the shRNA were selected using puromycin (4 μg/mL) (Sigma-Aldrich). All cell lines tested negative for Mycoplasma.
Proliferation, apoptosis and cell cycle assays in vitro
To study proliferation, cell death and cell cycle, B16 and HCT-116 cells were cultured until reaching 70% confluency and then stimulated with DEX (200 nM) or forskolin (FSK) (100 nM). Medium was replaced after 2 h. In different experiments, the cells were exposed to a heat shock of 43 °C for 30 min . Live and dead cells were counted using Trypan blue, and apoptotic cells were assessed by Annexin V staining. Cell cycle phases were studied by bromodeoxyuridine (BrdU) and 7-aminoactinomycin D (7AAD) stainings, cell cycle phase distribution and cell cycle arrest were measured by Ki67 and Annexin V stainings, and mitotic index was assessed by phospho-histone H3 (pHH3) staining, using standard protocols. More details can be found in Additional file 2.
Animals, DEX injections and tumor growth monitoring
C57BL/6J mice and NSG mice (Jackson Laboratories, Bar Harbor, ME, USA) were housed (≤5/cage) under 12 h light (100 lux):12 h dark (0 lux) conditions with food and water available ad libitum. Male mice (2–3 months old) were used in all experiments, except for one experiment with shRNA-expressing tumors to evaluate the tumor growth, in which 4-month-old females were used. The sample size of all biological replicates per time point is indicated in each figure legend or related supplementary table and mice were randomized between all groups.
C57BL/6J mice or NSG mice were inoculated with 1.5 × 106 B16 cells in the tail vein or subcutaneously or 3 × 106 HCT-116 cells. The s.c. tumor volume was measured in two dimensions with a caliper and calculated based on the volume of an ellipsoid. When s.c. tumors reached a volume of ~100 μL (after 10–15 days), DEX (or PBS) was injected intra-tumorally every second day at Zeitgeber Time (ZT) 6 (6 hours after lights on) to reach a concentration of 200 nM within the tumor (calculated based on the tumor volume). Tumor growth was measured daily. Tumor growth was compared showing absolute tumor volume when the tumors were on average 100 μL and did not differ between mice by more than approximately ±15 μL at the first treatment day. In case of experimental starting conditions when the tumor volume of mice differed more than 50 μL between individual mice at the first treatment day, the relative tumor growth was calculated relative to the initial starting volume for each individual mouse. Mice were killed by cervical dislocation at the indicated circadian times (CTs) during the second day of darkness, 18–25 days after inoculation. Eyes were removed under a 15 W red safety light prior to dissection. Tumors and host organs were harvested and kept at −80 °C until further analysis.
Cell cycle, immune cell labeling and protein expression assays on tumors
Cell cycle phases were determined using BrdU and 7AAD staining. BrdU (1.2 mg/ml) was injected intra-tumorally 6 h before tumors were collected. Cell lysates from fixed s.c. tumors were incubated with mouse anti-BrdU antibody and then with Alexa Fluor 488 goat anti-mouse IgG. Finally, cells were incubated with 7AAD viability staining solution. Mitotic index was evaluated on tumor cell lysate incubated with anti-pHH3 antibody and then with Alexa Fluor 488 donkey anti-rabbit antibody. A second set of cell lysates were stained for Annexin V. Cell cycle arrest and proliferation was detected in cells from fixed s.c. tumors in NSG mice or in Scrambled shRNA and Bmal1 shRNA cultured cells using the Ki67 Set according to manufacturer’s protocol.
For tumor immune cell infiltration in vivo, tumors were collected throughout the circadian day (second day in darkness) on the seventh day after the first DEX treatment. One million cells from s.c. tumor suspensions with and without collagenase treatment were blocked with Fc Block and then incubated with first antibodies for T cells (CD4, CD8), B cells (CD19), dendritic cells (CD11c), macrophages (F4/80, CD11b), neutrophils (CD11b, F4/80, Ly6G) or monocytes (CD11b, F4/80, Ly6C), followed by labeled streptavidin in the case of CD11b staining.
For protein expression in vivo, tumors were collected (as described above) and fixed in 4% paraformaldehyde, permeabilized with 90% methanol, and incubated with antibodies for WEE1, c-MYC, CYCLIN E (CCNE), CDK2, p57 (CDKN1c), CDK1, p21 (CDKN1a) or BMAL1 (ARNTL). After blocking with 10% rat or goat serum, appropriate secondary antibodies were used. Controls for each sample were stained with the secondary antibody alone. Finally, the cell suspensions were analyzed by flow cytometry.
All samples were analyzed by flow cytometry using a FACS Calibur (BD Biosciences, San Jose, CA, USA) and FlowJo software (FlowJo, LLC, Ashland, Oregon, USA). Controls for each sample were stained with the secondary antibody alone. More details can be found in Additional file 2, including panel descriptions, antibodies and fluorophores.
Quantitative polymerase chain reaction and immunohistochemistry
Standard protocols were used to perform quantitative polymerase chain reaction (PCR) and immunohistochemistry. Details about protocols, primer sequences, antibodies and data analysis can be found in Additional file 2.
Statistical analyses were done with GraphPad Prism (GraphPad Software, San Diego, CA, USA). Mann-Whitney rank sum test (alpha = 0.05, two-tailed) was used for knockdown efficiency. Circadian variation was tested by fitting a cosine-wave equation,
on clock gene expression or a double harmonic cosine-wave equation,
on cell cycle gene expression data, with a fixed 24-h period; significance was determined using an F-test. For datasets with more than two time points, a Kruskal-Wallis test was used (alpha = 0.05, two-tailed), taking the small sample size into consideration even if the normality test passed. For differences over time between two groups or more, two-way ANOVA was used, followed by Bonferroni’s posthoc test. A statistically significant difference was assumed when p < 0.05. Statistical details are presented in Additional file 1.
Induction of circadian clock function in B16 melanoma cells
First we characterized circadian rhythm generation in B16 melanoma cells. Reporter constructs consisting of the luciferase gene under the control of the Bmal1 or the Per2 promoter (Bmal1-Luc, Per2-Luc) were stably transfected in B16 cells. The bioluminescence of these cells was arrhythmic (Fig. 1a, from −44 to 0 h). However, upon addition of DEX, an agonist of the glucocorticoid receptor (which is expressed in B16 cells ) known to induce circadian rhythms in cultured cells, we observed rhythmic Bmal1-Luc and Per2-Luc promoter activity with the expected opposite phases (Fig. 1a) , which, however dampened earlier than in various non-cancer cell lines [35, 36].
To address whether the loss of rhythmicity after a few cycles resulted from circadian dysfunction in individual cells or from a desynchronization among rhythmic cells, we analyzed Per2-Luc bioluminescence at the single-cell level (Fig. 1b, Additional file 3, Additional file 4A–E). Although rhythms in the circadian range (first to second peak: 24.2 ± 1.4 h, second to third peak: 25.3 ± 2.0 h, third to fourth peak: 24.3 ± 1.5 h; Additional file 4E, F) were induced by DEX in ~90% of the cells, they quickly dampened within two to three cycles: 50% and 36% of the cells showed a second or third circadian peak, respectively, but circadian rhythms in bioluminescence were greatly suppressed in all cells after 132 h (Fig. 1b, Additional file 4A–D, G). Similarly the amplitude of single-cell rhythms dropped by about 80% within three cycles and the phase distribution became dispersed after 48 h (Additional file 4H, I). Repeated treatments showed that clock gene suppression was not due to cell death (Additional file 4J). Overall, these data indicated a suppression of clock gene expression in B16 cells rather than a desynchronization between single cells.
Rhythmic clock gene expression was also observed when employing alternative methods for clock gene activation [30, 37]: FSK, an activator of adenylyl cyclase and of the cAMP/PKA pathway (Fig. 1c), heat shock (Fig. 1d) and serum shock (Fig. 1e) all induced transcript oscillations in B16 cells. In addition to Bmal1 and Per2, the mRNAs of clock genes Per1, Cry1 and Nr1d1 also fluctuated rhythmically in B16 cells after DEX treatment but not in untreated cells (Fig. 1f–j).
Altogether, these results indicated that the B16 cells harbor an unstable but inducible circadian oscillator. We decided to take advantage of this property to address the role of the tumor cell-intrinsic clock in cell proliferation and tumor growth.
The cell cycle is under circadian control after dexamethasone treatment in vitro
Because the molecular clockwork was shown to regulate the expression of genes encoding cell cycle regulators , we set out to study the expression of such genes in B16 cells. B16 cells were treated with DEX for 2 h, harvested over 24 h, and tested for mRNA expression of WEE 1 homolog 1 (Wee1), Cyclin-dependent kinase 1 (Cdk1), Cdk2, Cyclin E, Myelocytomatosis oncogene c (c-Myc) and Cyclin-dependent kinase inhibitor 1A (p21). All six genes showed predominant 24-h rhythm components in transcript abundance as a consequence of DEX treatment (Fig. 1k–p).
Because these factors are involved in cell cycle checkpoints, we assessed the effect of DEX treatment on the distribution of B16 cells among cell cycle stages. Cells were collected at different time points over 24 h, stained for BrdU incorporation and with 7AAD, and analyzed by flow cytometry (Fig. 2a, b). The proportion of cells in G0/1, G2/M and S phases was found to be rhythmic in cells treated with DEX, while control cells showed no circadian variation (Fig. 2c–e). Interestingly, fewer cells entered the S phase 24, 36 and 42 h after DEX treatment (Fig. 2e), indicating less DNA replication, while more cells were found in G0/G1 phases (Fig. 2c).
Induction of the circadian clock slows down B16 cell proliferation in vitro
Given that activation of the circadian clock in B16 cells triggered rhythms of cell cycle genes and phases, we next tested whether activation of the clock in B16 cells influences their proliferation. Thirty-six hours after DEX treatment, we counted significantly fewer live cells than without treatment (Fig. 2f), while the amount of dead cells in the medium was unchanged after 12–48 h (Additional file 4N). The effect was even more pronounced after 2 days, with ~50% fewer live cells but similar numbers of dead cells after DEX treatment (Fig. 2g, Additional file 4O). Of note, the numbers of live and dead cells were similar before and immediately after the end of the 2 h DEX treatment, suggesting that the treatment did not acutely induce cellular toxicity (Additional file 4K).
Because rhythms quickly dampened after treatment (Fig. 1) we tested whether repeated DEX treatment could further inhibit cell proliferation. While a single DEX treatment significantly reduced cell numbers after 50 h, a second treatment further reduced the amount of cells after 96 h (Fig. 2h). Population doubling time (PDT) was increased to 22.7 h in single DEX-treated cells and further to 23.0 h in double DEX-treated cells compared to 16.5 h PDT in untreated control cells. Annexin V staining indicated that the differences in cell counts were not due to differences in levels of apoptosis (Additional file 4P). Total cell numbers were even more reduced after three DEX treatments administered every 48 h (Additional file 4L, M).
Similar experiments were also conducted with other stimuli activating the B16 clock (Fig. 1). Both a single FSK treatment (Fig. 2f, g) and repeated FSK treatments (Additional file 4M) were as effective as DEX in slowing down B16 cell proliferation. Also, FSK treatment did not affect cell death rates (Additional file 4N, O), nor did it acutely impact on cell numbers right after the 2 h treatment (Additional file 4K). Moreover, exposing the cells to a 30 min heat shock was sufficient to reduce proliferation without affecting apoptosis (Fig. 2i, Additional file 4Q). PDT was increased to 20.7 h after heat shock compared to 17.2 h in untreated cells. These data suggested that the reduction in cell proliferation might be due to action on intrinsic clock function, as activating clock gene expression was the common denominator of all three treatments.
Dexamethasone activates the circadian clock in B16 tumors
B16 melanoma cells, which represent a well-established and widely used mouse model for human melanoma , form lung and s.c. tumors when injected in the tail vein and subcutaneously, respectively (Additional file 5A, B). The analysis of circadian clock gene expression in B16 lung tumors unveiled suppressed or arrhythmic Per1, Per2 and Bmal1 expression, while there was robust circadian oscillation in the neighboring lung tissue (Fig. 3a). Similarly, Per1, Per2, Bmal1 and Nr1d1 expression was arrhythmic in s.c. B16 tumors (Fig. 3b).
DEX, an agonist of the glucocorticoid receptor, is well known to reset cellular clocks by inducing Per gene expression . Upon repeated addition of DEX, we observed rhythmic Bmal1-Luciferase reporter expression in slice cultures of explanted B16 lung tumors (Fig. 3c). Moreover, monitoring of single cells within the same lung tumor slice indicated an absence of Bmal1 rhythms before treatment, but circadian oscillation of Bmal1 after DEX treatment (Additional file 6, Fig. 3d). Thus, DEX induces de novo rhythmic Bmal1 gene expression in single B16 cells rather than synchronizing cellular oscillators. This is consistent with the single-cell data obtained on B16 cells in vitro (Fig. 1, Additional files 3 and 4).
To further confirm an activation of the tumor clock by DEX in vivo, s.c. tumors were injected intra-tumorally with DEX every 48 h to ensure maintenance of tumor clock activation. Rhythmic clock gene expression in tumors was found after DEX but not PBS treatment (Fig. 3e–i). Per1, Per2, Cry1 and Nr1d1 expression showed a significant effect of time and treatment. Rhythmicity of Bmal1 mRNA expression did not reach significance (Fig. 3i). However, the ANOVA analysis showed an effect of time (see Additional file 1), and immunohistochemistry on s.c. tumor slices revealed a significant rhythm of BMAL1 protein levels in DEX-treated tumors, but not in PBS-treated tumors (Fig. 3j, Additional file 5C, D).
The efficiency and specificity of the intra-tumoral injections were evaluated by injecting methylene blue in tumors. The injected fluid spanned the whole tumor tissue 6 h after intra-tumoral injection, but was absent in surrounding tissues (Additional file 5E). To further assess the specificity of the response, clock gene expression in the liver - a non-cancerous, peripheral tissue - was compared between PBS- and DEX-injected mice: we found no significant differences between the treatment groups (Additional file 5F).
Altogether, these results indicated that the B16 tumors harbor a suppressed but inducible circadian oscillator. Moreover, these experiments showed that repeated DEX injection consistently induced rhythmic clock gene expression in B16 tumors rather than re-synchronized them. The ability to compare the B16 tumors with or without circadian clock function gave us the opportunity to test the role of the tumor-intrinsic clock in regulating cell cycle and tumor growth.
The cell cycle is under circadian control after dexamethasone treatment of B16 tumors
We measured the expression of cell cycle regulators in s.c. B16 tumors harvested over 24 h. Similar to the data obtained in vitro (Fig. 1k–p), rhythmic protein expression of CYCLIN E, p21 and c-MYC was found in DEX-treated tumors, but not in PBS-treated tumors (Fig. 4a–c, Additional file 7A–C). On the other hand, WEE1, CDK1, CDK2 and p57, a direct glucocorticoid receptor target , did not show a daily variation in the DEX-treated tumors (Fig. 4d–g).
Homogenized tumor cells collected at different time points were stained for BrdU incorporation and with 7AAD. The proportion of cells in G0/1 and S phases was found to be rhythmic in DEX-treated control tumors, whereas PBS-treated tumors showed no circadian variation (Fig. 4h–j, Additional file 7D). Interestingly, fewer rhythmic cells entered the S phase in DEX-treated tumors, indicating less DNA replication, whereas more cells were found in G0/G1 phases. Importantly, DEX treatment reduced rather than increased the number of cells in G0 arrest as indicated by Ki67/7AAD staining in vitro (see control cells in Additional file 8). Consistent with results obtained from BrdU stainings, cell numbers in G1 phase were increased, while cells distributed in S/G2/M phases were slightly reduced (compare Figs. 2 and 4 and Additional file 8). Thus, reduced cell numbers after DEX treatment were not caused by cell cycle arrest. Moreover, even though entrance to G2/M phase was not rhythmically controlled in the tumor, mitotic index assessed by pHH3 staining indicated a rhythmic percentage of cells undergoing mitosis (Fig. 4k, Additional file 7E). Interestingly, cells from DEX-treated tumors underwent apoptosis in a circadian manner (Fig. 4l, Additional file 7F).
Dexamethasone treatment slows down B16 tumor growth
Given that activation of the circadian clock in B16 tumors triggered rhythms of cell cycle genes and phases, we then evaluated whether the activation of clock function in B16 tumors was paralleled by a reduction in tumor growth. To this end, s.c. B16 tumor growth was compared between DEX- and PBS-treated tumors. DEX treatment significantly slowed down tumor growth (by ~60% after 8 days) compared to PBS treatment (Fig. 4m). Importantly though, Annexin V staining indicated that the differences in tumor growth were not due to differences in the levels of apoptosis, because a similar proportion of apoptotic cells were found in DEX- and PBS-treated tumors (when averaged over the 24-h day, PBS: 14.6 ± 2.3% versus DEX: 11.5 ± 4.6, extra sum-of squares F-test: p = 0.25; Fig. 4l).
To rule out that reduced tumor growth after DEX treatment may be caused by DEX-induced immune cell infiltration in the tumor, we repeated this experiment in immune-deficient NSG mice, which lack T cells, B cells and natural killer cells. Similarly to results in C57BL/6J hosts, tumor growth was strongly reduced by DEX in NSG mice (Fig. 4n), and no differences were found in the levels of infiltration of remaining immune cells between DEX- and PBS-treated tumors in NSG mice (Additional file 9A–C). Again, the proportion of cells undergoing apoptosis was not significantly different between DEX- and PBS-treated tumors collected at Circadian Time (CT)14 in NSG mice (Additional file 9D). Moreover, the proportions of cells undergoing cell division (G1/S/G2/M) and of those in G0 arrest were unchanged by DEX treatment of tumors in NSG mice (Additional file 9E). Together with results obtained in vitro that excluded cell cycle arrest (Additional file 8A) and in C57BL/6J mice that showed more cells in G0/G1 phase at CT14 upon DEX treatment, these results indicated that cells remain more in G1 phase and transit less to the S phase.
Knockdown of Bmal1 abolishes the effects of dexamethasone on clock genes and cell cycle genes
To test whether the activation of the clock in B16 tumors is the causal link between DEX treatment and the inhibition of tumor growth, experiments were repeated in B16 tumors with a disrupted circadian clock. Using a lentiviral vector, we stably introduced into B16 cells an shRNA against Bmal1, a necessary component of the circadian clock . Bmal1 shRNA-transfected cells expressed ~80% less Bmal1 RNA and ~65% less BMAL1 protein than Scrambled shRNA control cells (Fig. 5a, b). B16 cells stably expressing shRNA against Bmal1 or Scrambled shRNA were injected subcutaneously into mice to form either tumors lacking a functional clock or control tumors. Similarly to non-transfected tumors, clock gene expression showed significant circadian rhythms in DEX-treated but not PBS-treated Scrambled shRNA tumors (compare Fig. 3 and Fig. 5c–g). In Bmal1 shRNA tumors, Bmal1 expression was reduced by ~70% in both DEX- and PBS-treated tumors (Fig. 5c). Accordingly, the expression of BMAL1 target genes Per1, Per2, Cry1 and Nr1d1 was suppressed and arrhythmic, indicating effective disruption of the clock machinery in the tumors (Fig. 5d–g). Thus, Bmal1 knockdown completely prevented the induction of circadian rhythms by DEX in the Bmal1 shRNA tumors.
Rhythmic gene expression of Cyclin E, p21 and c-Myc was only found in DEX-treated Scrambled shRNA tumors; Cdk1, Cdk2 and Wee1 did not show a daily variation, in line with cell cycle protein data (compare Fig. 5h–m and Fig. 4a–f). Importantly, abrogation of DEX-induced activation of the circadian clock in Bmal1 shRNA tumors was reflected by the arrhythmic expression of cell cycle genes in these tumors. Consistently, Bmal1 knockdown in vitro also prevented the DEX-induced rhythms in cell cycle phases (Additional file 8A–E).
Knockdown of Bmal1 prevents the inhibitory effect of dexamethasone on tumor growth
Next we sought to determine whether clock function in the B16 tumors is needed for DEX-induced reduction in tumor growth. As expected, B16 tumors expressing the Scrambled shRNA grew more slowly during DEX treatment: after 7 days, DEX-treated tumors were ~60% smaller than PBS-treated tumors (Fig. 5n) and this is consistent with the growth of untransfected tumors (Fig. 4m, n). In contrast, tumor volumes were indistinguishable between DEX- and PBS-treated mice harboring Bmal1 shRNA tumors (Fig. 5n). Thus, DEX had no effect on tumor growth after Bmal1 knockdown. Volume doubling time analysis of Scrambled and Bmal1 shRNA tumors confirmed these results (Scrambled shRNA: PBS: 53.3 h, DEX: 84.0 h; Bmal1 shRNA: PBS: 50.1 h, DEX: 50.0 h). Similar results were obtained in vitro using Bmal1 and Scrambled shRNA-transfected cells (data not shown).
Consistent with the data obtained using NSG mice (Fig. 4n), DEX did not affect the levels of immune cell infiltration in B16 tumors inoculated in the syngeneic C57BL/6J mice or in Bmal1 knockdown tumors, indicated by similar values for B cells, dendritic cells, CD4+ and CD8+ T cells, macrophages, neutrophils, and monocytes (Additional file 8F–L). These data confirmed that the slower tumor growth was not caused by effects of DEX on immune cell infiltration. Overall, these findings are in strong support of the notion that activating circadian clock function within B16 tumors slows down their growth.
Enhancement of circadian rhythms slows down HCT-116 tumor growth
To test the link between the circadian clock and tumor growth beyond our model using mouse melanoma, we treated human HCT-116 colon carcinoma cells with DEX and measured clock gene expression as well as proliferation and apoptosis up to 48 h after the treatment. HCT-116 cells exhibited rhythmic clock gene expression upon DEX treatment (Fig. 6a, b), which could be due to either synchronization of individual cells’ clocks or de novo activation of clocks in the cells. Upon this treatment HCT-116 cell proliferation was strongly decreased while apoptosis levels were unaffected (Fig. 6c, d).
Similar to the B16 s.c. tumors in C57BL/6 J and NSG mice, growth of tumors formed in NSG mice after HCT-116 cell inoculation was strongly slowed down after DEX treatment (Fig. 6e). These data underscore the possibility that controlling cell division rate by circadian clock enhancement and thus controlling tumor growth is not restricted to mouse melanoma cells, and may be generally applicable to human cancer cells and to other cancer types.
In this report, we showed that B16 melanoma cells and B16 tumors have suppressed expression of clock components, which is in line with previous reports on different cancer cell lines and tumors [21–23]. However, we discovered that different treatments could restore clock gene expression in B16 cells and tumors. This provided an experimental model in which the same tumor type could be compared in conditions of inactive or active circadian oscillator function. Using this model, we showed that restoring clock function in B16 melanoma cells strongly reduced cell proliferation in vitro and tumor growth in vivo (Fig. 7). We also extended our observations to another cancer cell model, the human colon carcinoma HCT-116 cells. In all of the in vivo tumor experiments, a strong slowdown of tumor growth was observed, with a two thirds reduction of tumor size after 8 days of treatment, regardless of the host or cancer cell line used.
The amplitude of clock gene rhythmicity within tumors was previously correlated with their growth in mice bearing Glasgow osteosarcoma  and pancreatic adenocarcinoma . Furthermore, a dysregulated circadian tumor clock in human patients correlated with their prognosis [25, 41]. Together, these prior studies indicate that the tumor clock may have an impact on tumor growth and overall survival (also reviewed in ). However, until our present report, a causal link was missing to solidify the importance of the tumor clock itself, as opposed to host-derived circadian rhythms. Previous studies showed that glucocorticoids suppress proliferation in human melanoma cells and B16 tumors after intraperitoneal DEX injection in mice [28, 43]. Importantly, our data provide a cellular mechanism for these effects. In contrast to prior work, our data were generated using intra-tumor injection of DEX restricted to the tumor and at low doses. Furthermore, we showed an absence of effects on clock gene expression in the liver. Thus, our work is the first to show a tumor-intrinsic mechanism for the control of tumor growth by the circadian clock. Moreover, the effects of restored synchronous circadian rhythmicity on tumor growth also extend to a distinct tumor cell model, the human colon carcinoma HCT-116 cells, although in the case of these cells we cannot exclude a role of DEX in synchronizing the clocks in individual cells rather than an activation of the cellular clocks.
DEX and FSK have previously been reported to have varying effects on apoptosis, depending on the cell line or tumor model used [44–47]. Nevertheless, and in line with previous reports on fibroblasts , we found no or minor effects of DEX, FSK or heat shock on apoptosis in B16 cells. Thus, in our experiments, the activation of circadian clock function in tumors resulted in reduced growth independently of deregulated apoptosis. Given the immune-modulating properties of glucocorticoids , we also aimed to exclude an effect of DEX on the immune cell content of the tumors as the cause of the observed decrease in tumor growth. Notably, immune cell content was not changed by the intra-tumoral DEX treatment. Moreover, the effect of DEX on tumor growth was recapitulated in NSG mice, which lack T cells, B cells and natural killer cells, further strengthening our claim. In order to directly test the hypothesis that DEX inhibits tumor growth via the tumor-intrinsic circadian clock, we used shRNA against the essential clock gene Bmal1. The response to DEX was abrogated in B16 tumors with a Bmal1 knockdown. Thus, the suppressive DEX effect on B16 proliferation and tumor growth requires a functional clock within B16 cells. It is unlikely that Bmal1 knockdown affects the response to DEX itself, because Bmal1 dysfunction did not interfere with glucocorticoid receptor expression as observed in transcriptome datasets [49–51]. Of note, we observed a similar induction of circadian rhythms and inhibition of B16 cell proliferation in vitro following other treatments besides DEX, as well as with a non-pharmacological treatment, heat shock. Serum, DEX, FSK and heat shock all reset cellular clocks by inducing clock genes such as Per genes [30, 39, 52], but different signaling pathways are involved: DEX activates Per1 via the glucocorticoid receptor , but DEX can also synchronize the circadian clock via glucocorticoid receptor-independent pathways, as was shown for HCT-116 cells ; FSK activates the cAMP/protein kinase A pathway, and thus, cAMP response element-binding protein activity at the Per1 promoter ; and heat shock activates Per2 transcription via heat shock factor 1 . Given that these treatments similarly activate the clock by mechanisms distinct from DEX, this further suggests a clock-dependent action of DEX.
Taken together our results indicate that reduced tumor growth after DEX treatment was not caused by enhanced apoptosis, nor immune infiltration in the tumor, but rather relies specifically on inducing circadian rhythms within the tumor. For the first time, our work unveils a causal relationship between the tumor-intrinsic circadian clock and tumor growth (Fig. 7).
Our findings raise the question of how the activation of circadian clock function in B16 cells leads to inhibition of tumor growth. The circadian clock has been shown to regulate cell cycle genes and, thus, progression through the cell cycle . Indeed, we identified rhythmic cell cycle genes after induction of clock function in B16 cells and tumors. In particular, Cyclin E, p21 and c-Myc exhibited circadian oscillations at the mRNA and protein levels. CLOCK-BMAL1 represses c-Myc, an activator of Cyclin E [16, 55], and another clock component, NR1D1, inhibits the synthesis of the CDK inhibitor p21 . Thus, restored expression of the major clock components in B16 tumors likely accounts for the observed changes in cell cycle gene expression.
Our data indicate that the circadian gating distributes more B16 cells in the G1 phase (and not more arrest of cells in the G0 phase) and fewer in the S phase, which prolongs the transit through the cell cycle and may account for the observed lengthening of the PDT. Thus, fewer cells initiated DNA replication, which could underlie the observed reduced tumor growth. In line with our observations, accumulation in cell cycle phases such as G1 or G2 was reported to slow down proliferation in human melanoma cells . G1-to-S transit is regulated by cell cycle checkpoint regulators, in particular the Cyclin E/CDK2 complex . Importantly we have identified rhythmic expression of the inhibitor p21, c-MYC and a component of this checkpoint complex itself, Cyclin E. Consequently, rhythmic regulation of the Cyclin E/Cdk2 complex may result in a prolonged stay in the G1 phase. Taken together, rhythmic changes in expression levels of Cyclin E, p21 and c-MYC after activation of the clock by DEX likely caused the observed redistribution of B16 cells among cell cycle phases (Fig. 7). Moreover, our results highlight a possible strategy of B16 melanoma cells to facilitate their proliferation: suppression of the circadian clock induces changes in their cell cycle, which leads to increased residence time in the S phase and an enhancement of DNA replication and thus cell proliferation.
Glucocorticoids have been used to treat various cancer types for decades, in many cases as an adjuvant to other chemotherapies . While potential mechanisms have been described in different cell types, exactly how glucocorticoids regulate apoptosis or cell cycle progression is not fully understood [59, 60]. Our work indicates a possible mechanism (capable of explaining existing data) for how glucocorticoids can inhibit cancer cell proliferation, namely by inducing circadian rhythms in cancer cell cycle events to limit the number of cells in the S phase and thereby increase the time spent in the G1 phase. Therefore, our work opens new windows of opportunity in cancer therapy based on chronobiological intervention. For example, activation of the clock in tumors may represent a new therapeutic target for malignant melanoma therapy in humans. Because our observations extended to human colon cancer cells, this strategy might more generally become an innovative way to slow down cancer progression and thereby improve the outcome of established anti-cancer therapies. Slowing down tumor progression by improving circadian rhythmicity might critically delay cancer progression and/or metastasis. This could in turn increase treatment success with traditional chemotherapy or provide a broader time window for surgical resection of tumors.
Bernard S, Herzel H. Why do cells cycle with a 24 hour period? Genome Inform. 2006;17(1):72–9.
Masri S, Cervantes M, Sassone-Corsi P. The circadian clock and cell cycle: interconnected biological circuits. Curr Opin Cell Biol. 2013;25(6):730–4.
Levi F, Schibler U. Circadian rhythms: mechanisms and therapeutic implications. Annu Rev Pharmacol Toxicol. 2007;47:593–628.
Duguay D, Cermakian N. The crosstalk between physiology and circadian clock proteins. Chronobiol Int. 2009;26(8):1479–513.
Zhang R, Lahens NF, Ballance HI, Hughes ME, Hogenesch JB. A circadian gene expression atlas in mammals: implications for biology and medicine. Proc Natl Acad Sci U S A. 2014;111(45):16219–24.
Cermakian N, Lange T, Golombek D, Sarkar D, Nakao A, Shibata S, et al. Crosstalk between the circadian clock circuitry and the immune system. Chronobiol Int. 2013;30(7):870–88.
Hansen J. Increased breast cancer risk among women who work predominantly at night. Epidemiology. 2001;12(1):74–7.
Haus EL, Smolensky MH. Shift work and cancer risk: potential mechanistic roles of circadian disruption, light at night, and sleep deprivation. Sleep Med Rev. 2012;17(4):273–84.
Kloog I, Haim A, Stevens RG, Portnov BA. Global co-distribution of light at night (LAN) and cancers of prostate, colon, and lung in men. Chronobiol Int. 2009;26(1):108–25.
Lahti TA, Partonen T, Kyyronen P, Kauppinen T, Pukkala E. Night-time work predisposes to non-Hodgkin lymphoma. Int J Cancer. 2008;123(9):2148–51.
Filipski E, Innominato PF, Wu M, Li XM, Iacobelli S, Xian LJ, et al. Effects of light and food schedules on liver and tumor molecular clocks in mice. J Natl Cancer Inst. 2005;97(7):507–17.
Logan RW, Zhang C, Murugan S, O’Connell S, Levitt D, Rosenwasser AM, et al. Chronic shift-lag alters the circadian clock of NK cells and promotes lung cancer growth in rats. J Immunol. 2012;188(6):2583–91.
Filipski E, Levi F. Circadian disruption in experimental cancer processes. Integr Cancer Ther. 2009;8(4):298–302.
Miyazaki K, Wakabayashi M, Hara Y, Ishida N. Tumor growth suppression in vivo by overexpression of the circadian component, PER2. Genes Cells. 2010;15(4):351–8.
Zeng ZL, Wu MW, Sun J, Sun YL, Cai YC, Huang YJ, et al. Effects of the biological clock gene Bmal1 on tumour growth and anti-cancer drug activity. J Biochem. 2010;148(3):319–26.
Fu L, Pelicano H, Liu J, Huang P, Lee C. The circadian gene Period2 plays an important role in tumor suppression and DNA damage response in vivo. Cell. 2002;111(1):41–50.
Lee S, Donehower LA, Herron AJ, Moore DD, Fu L. Disrupting circadian homeostasis of sympathetic signaling promotes tumor development in mice. PLoS One. 2010;5(6), e10995.
Mteyrek A, Filipski E, Guettier C, Okyar A, Levi F. Clock gene Per2 as a controller of liver carcinogenesis. Oncotarget. 2016;7(52):85832–47.
Bieler J, Cannavo R, Gustafson K, Gobet C, Gatfield D, Naef F. Robust synchronization of coupled circadian and cell cycle oscillators in single mammalian cells. Mol Syst Biol. 2014;10:739.
Feillet C, van der Horst GT, Levi F, Rand DA, Delaunay F. Coupling between the circadian clock and cell cycle oscillators: implication for healthy cells and malignant growth. Front Neurol. 2015;6:96.
Relogio A, Thomas P, Medina-Perez P, Reischl S, Bervoets S, Gloc E, et al. Ras-mediated deregulation of the circadian clock in cancer. PLoS Genet. 2014;10(5), e1004338.
Iurisci I, Filipski E, Reinhardt J, Bach S, Gianella-Borradori A, Iacobelli S, et al. Improved tumor control through circadian clock induction by Seliciclib, a cyclin-dependent kinase inhibitor. Cancer Res. 2006;66(22):10720–8.
Li XM, Delaunay F, Dulong S, Claustrat B, Zampera S, Fujii Y, et al. Cancer inhibition through circadian reprogramming of tumor transcriptome with meal timing. Cancer Res. 2010;70(8):3351–60.
Innominato PF, Levi FA, Bjarnason GA. Chronotherapy and the molecular clock: clinical implications in oncology. Adv Drug Deliv Rev. 2010;62(9-10):979–1001.
Oshima T, Takenoshita S, Akaike M, Kunisaki C, Fujii S, Nozaki A, et al. Expression of circadian genes correlates with liver metastasis and outcomes in colorectal cancer. Oncol Rep. 2011;25(5):1439–46.
Teicher BA. Tumor models in cancer research. 2nd ed. Totowa: Humana Press; 2002.
Brattain MG, Fine WD, Khaled FM, Thompson J, Brattain DE. Heterogeneity of malignant cells from a human colonic carcinoma. Cancer Res. 1981;41(5):1751–6.
Crowley P, Lai NY, De Young N, Pearce P, Funder JW, Gill PG. Inhibition of growth of B16 melanoma by glucocorticoids does not result directly from receptor-mediated inhibition of tumour cells. Oncology. 1988;45(4):331–5.
Fiszer-Kierzkowska A, Vydra N, Wysocka-Wycisk A, Kronekova Z, Jarzab M, Lisowska KM, et al. Liposome-based DNA carriers may induce cellular stress response and change gene expression pattern in transfected cells. BMC Mol Biol. 2011;12:27.
Tamaru T, Hattori M, Honda K, Benjamin I, Ozawa T, Takamatsu K. Synchronization of circadian Per2 rhythms and HSF1-BMAL1:CLOCK interaction in mouse fibroblasts after short-term heat shock pulse. PLoS One. 2011;6(9), e24521.
Ichijo T, Chrousos GP, Kino T. Activated glucocorticoid receptor interacts with the INHAT component Set/TAF-Ibeta and releases it from a glucocorticoid-responsive gene promoter, relieving repression: implications for the pathogenesis of glucocorticoid resistance in acute undifferentiated leukemia with Set-Can translocation. Mol Cell Endocrinol. 2008;283(1-2):19–31.
Zhu XY, Liu YJ, Diao F, Fan J, Lu J, Xu RB. Role of glucocorticoids and glucocorticoid receptor in priming of macrophages caused by glucocorticoid receptor blockade. Endocrine. 2007;31(2):130–7.
Sherman H, Froy O. Expression of human beta-defensin 1 is regulated via c-Myc and the biological clock. Mol Immunol. 2008;45(11):3163–7.
Yan J, Wang H, Liu Y, Shao C. Analysis of gene regulatory networks in the mammalian circadian rhythm. PLoS Comput Biol. 2008;4(10), e1000193.
Nagoshi E, Saini C, Bauer C, Laroche T, Naef F, Schibler U. Circadian gene expression in individual fibroblasts: cell-autonomous and self-sustained oscillators pass time to daughter cells. Cell. 2004;119(5):693–705.
Welsh DK, Yoo SH, Liu AC, Takahashi JS, Kay SA. Bioluminescence imaging of individual fibroblasts reveals persistent, independently phased circadian rhythms of clock gene expression. Curr Biol. 2004;14(24):2289–95.
Balsalobre A, Damiola F, Schibler U. A serum shock induces circadian gene expression in mammalian tissue culture cells. Cell. 1998;93(6):929–37.
Overwijk WW, Restifo NP. B16 as a mouse model for human melanoma. Curr Prot Immunol. 2001;Chapter 20:Unit 20.1.
Balsalobre A, Brown SA, Marcacci L, Tronche F, Kellendonk C, Reichardt HM, et al. Resetting of circadian time in peripheral tissues by glucocorticoid signaling. Science. 2000;289(5488):2344–7.
Rider CF, Shah S, Miller-Larsson A, Giembycz MA, Newton R. Cytokine-induced loss of glucocorticoid function: effect of kinase inhibitors, long-acting beta(2)-adrenoceptor [corrected] agonist and glucocorticoid receptor ligands. PLoS One. 2015;10(1), e0116773.
Chen ST, Choo KB, Hou MF, Yeh KT, Kuo SJ, Chang JG. Deregulated expression of the PER1, PER2 and PER3 genes in breast cancers. Carcinogenesis. 2005;26(7):1241–6.
Lévi F. Circadian clock induction. In: Schwab M, editor. Encyclopedia of Cancer. Berlin, Heidelberg: Springer Berlin Heidelberg; 2009. p. 691–4.
Osman AMM, Nasseir OA, Ismail NR. Potential mechanism for the effects of dexamethasone on growth of human melanoma cells in vitro. Health. 2010;2(8):857–61.
Hammer S, Sauer B, Spika I, Schraut C, Kleuser B, Schafer-Korting M. Glucocorticoids mediate differential anti-apoptotic effects in human fibroblasts and keratinocytes via sphingosine-1-phosphate formation. J Cell Biochem. 2004;91(4):840–51.
Petrella A, Ercolino SF, Festa M, Gentilella A, Tosco A, Conzen SD, et al. Dexamethasone inhibits TRAIL-induced apoptosis of thyroid cancer cells via Bcl-xL induction. Eur J Cancer. 2006;42(18):3287–93.
Thibaut S, Bourre L, Hernot D, Rousset N, Lajat Y, Patrice T. Effects of BAPTA-AM, Forskolin, DSF and Z.VAD.fmk on PDT-induced apoptosis and m-THPC phototoxicity on B16 cells. Apoptosis. 2002;7(2):99–106.
Valles SL, Benlloch M, Rodriguez ML, Mena S, Pellicer JA, Asensi M, et al. Stress hormones promote growth of B16-F10 melanoma metastases: an interleukin 6- and glutathione-dependent mechanism. J Transl Med. 2013;11:72.
Webster JI, Tonelli L, Sternberg EM. Neuroendocrine regulation of immunity. Annu Rev Immunol. 2002;20:125–63.
Bellet MM, Deriu E, Liu JZ, Grimaldi B, Blaschitz C, Zeller M, et al. Circadian clock regulates the host response to Salmonella. Proc Natl Acad Sci U S A. 2013;110(24):9897–902.
Guillaumond F, Becquet D, Boyer B, Bosler O, Delaunay F, Franc JL, et al. DNA microarray analysis and functional profile of pituitary transcriptome under core-clock protein BMAL1 control. Chronobiol Int. 2012;29(2):103–30.
Liu Y, Johnson BP, Shen AL, Wallisser JA, Krentz KJ, Moran SM, et al. Loss of BMAL1 in ovarian steroidogenic cells results in implantation failure in female mice. Proc Natl Acad Sci U S A. 2014;111(39):14295–300.
Balsalobre A, Marcacci L, Schibler U. Multiple signaling pathways elicit circadian gene expression in cultured Rat-1 fibroblasts. Curr Biol. 2000;10(20):1291–4.
Yamamoto T, Nakahata Y, Tanaka M, Yoshida M, Soma H, Shinohara K, et al. Acute physical stress elevates mouse period1 mRNA expression in mouse peripheral tissues via a glucocorticoid-responsive element. J Biol Chem. 2005;280(51):42036–43.
Travnickova-Bendova Z, Cermakian N, Reppert SM, Sassone-Corsi P. Bimodal regulation of mPeriod promoters by CREB-dependent signaling and CLOCK/BMAL1 activity. Proc Natl Acad Sci U S A. 2002;99(11):7728–33.
Perez-Roger I, Solomon DL, Sewing A, Land H. Myc activation of cyclin E/Cdk2 kinase involves induction of cyclin E gene transcription and inhibition of p27(Kip1) binding to newly formed complexes. Oncogene. 1997;14(20):2373–81.
Grechez-Cassiau A, Rayet B, Guillaumond F, Teboul M, Delaunay F. The circadian clock component BMAL1 is a critical regulator of p21WAF1/CIP1 expression and hepatocyte proliferation. J Biol Chem. 2008;283(8):4535–42.
Shapiro GI. Cyclin-dependent kinase pathways as targets for cancer treatment. J Clin Oncol. 2006;24(11):1770–83.
McKay LI, Cidlowski JA. Corticosteroids in the treatment of neoplasms. In: Kufe DW, Pollock RE, Weichselbaum RR, Bast J, Robert C, Gansler TS, Holland JF, et al., editors. Cancer Medicine. 6th ed. Hamilton ON: BC Decker; 2003.
Moutsatsou P, Papavassiliou AG. The glucocorticoid receptor signalling in breast cancer. J Cell Mol Med. 2008;12(1):145–63.
Schlossmacher G, Stevens A, White A. Glucocorticoid receptor-mediated apoptosis: mechanisms of resistance in cancer cells. J Endocrinol. 2011;211(1):17–25.
The authors thank the members of NC’s laboratory for discussions and technical help; Dr Hua Gu and Dr Dindial Ramotar for providing the B16 and HCT-116 cells, respectively; Dr Stephen Beesley for providing the plasmids and the luciferase reporter transfection protocol; Dr Gerardo Ferbeyre for advice and for providing the c-MYC and CDK2 antibodies; Dr El Bachir Affar for the CYCLIN E antibody; and Dr Shobhan Gaddameedhi for critical review of the manuscript.
This work was funded by a Canadian Institutes for Health Research grant (MOP-119322) (NC and NL), grants from Natural Sciences and Engineering Research Council (372813-2010) (Canada) and Canadian Foundation for Innovation (22740) (KFS), a Veterans Affairs Merit Award (1I01BX001146) (DKW), and a Fonds de recherche du Québec – Santé salary award (NC).
Availability of data and materials
All data generated or analyzed during this study are included in this published article (and its Additional files).
SK and NC conceived the project. SK and LBL performed experiments. SK analyzed most data. IDB, KFS designed and built the bioluminescent apparatus and analyzed the video data. DL analyzed the single-cell data. SK, DL, IDB, DKW, KFS, NL and NC provided critical intellectual input to the study and the manuscript preparation. SK and NC wrote the manuscript. All authors read and approved the final manuscript.
The authors declare that they have no competing interests.
Consent for publication
Ethics approval and consent to participate
Animal use was in accordance with the guidelines of the Canadian Council of Animal Care and was approved by the Douglas Institute Facility Animal Care Committee.
Supplementary tables. (PDF 362 kb)
Supplementary methods. (PDF 184 kb)
Single-cell analysis of Per2-Luc B16 cells and level of apoptosis after treatment. Bioluminescence of single Per2-Luc B16 cells after DEX treatment, grouped depending on their number of circadian peaks: (A) one peak (n = 19), (B) two peaks (n = 10), (C) three or more peaks (n = 9) and (D) abnormal and non-circadian peaks (n = 6). (E) Period distribution of single Per2-Luc B16 cells after DEX treatment. Analysis of circadian period (F), rhythmicity (G), amplitude (H) and peak time (I) of single Per2-Luc B16 cells. (J) Bioluminescence of Per2-Luc B16 cells undergoing repeated treatments (grey bars) after plating: medium change (day 1), DEX (day 4, 7) and FSK (day 10). (K) B16 cells were counted before, 2 h after treatment with DEX or FSK (untreated: n = 24, DEX: n = 6, FSK: n = 6, Kruskal-Wallis test, p > 0.05), (L) after a single or three DEX treatments and compared to untreated controls (n = 6 wells/time point, two-way ANOVA p < 0.001, posthoc test, *p < 0.05, ***p < 0.001 DEX1 compared to controls, +++ p < 0.001 DEX3 compared to controls, x p < 0.05 DEX1 compared to DEX3). (M) B16 cells were counted after a single or three DEX or FSK treatments and compared to untreated cells (control n = 25, DEX1: n = 16, DEX3: n = 4, FSK3: n = 4, Kruskal-Wallis test, Dunn’s multiple comparison test, **p < 0.01, ***p < 0.001). (N, O) Total dead cells in the medium 12–48 h (N) and 48–68 h (O) after treatment with either DEX or FSK and controls (n = 6–8 wells/time point). (P) Apoptotic cells stained for Annexin V 0–96 h after control or DEX treatment at 0 h (DEX1) or at 0 and 48 h (DEX2) (n = 4–12 wells/time point). (Q) Apoptotic cells stained for Annexin V 0–72 h after heat shock or control treatment (n = 6 wells/time point). Two-way ANOVA, posthoc test, ***p < 0.001 DEX compared to controls, +++ p < 0.001 FSK compared to controls. For details of statistics, see Additional file 1. (PDF 1581 kb)
B16 tumors and clock gene expression. (A) Lung tumors (black, indicated by arrows) formed after injection of 1.5 × 106 B16 cells in the tail vein, within the surrounding lung tissue (pink). (B) B16 tumors (black, indicated by arrow) formed after subcutaneous injection of 1.5 × 106 B16 cells in the neck. (C, D) Representative immunohistochemistry images for BMAL1 (green) and DAPI (blue) from PBS-treated (C) and DEX-treated (D) tumors collected at CT2, 8, 14 and 20. See full data in Fig. 3j. (E) Methylene blue (200 μL of 1% in saline) was injected intra-tumorally. Six hours later, tumors were harvested, sectioned and visualized by light microscopy. (F) Relative circadian clock gene expression in the liver of DEX- or PBS-treated mice harboring tumors generated by s.c. injection of B16 cells (n = 9–10, 2–3 mice/time point; cosine-wave regression, F-test: -DEX: Bmal1 and Nr1d1: p < 0.05, +DEX: Bmal1 and Cry1: p ≤ 0.01, Per1: p = 0.348, Per2: p = 0.174, Nr1d1: p = 0.0646; two-way ANOVA: group: all genes: p > 0.05, time: Bmal1, Per2, Cry1 and Nr1d1: p < 0.001; Per1: p < 0.01). Significant rhythms are illustrated with fitted cosine curves, otherwise data are connected by straight lines between data points, indicating no significant circadian rhythms. Data are represented as mean ± SEM. For details of statistics, see Additional file 1. (PDF 8 MB)
DEX induces rhythmic cell cycle protein expression and cell cycle phases, mitosis and apoptosis. Representative flow cytometry dot plots for p21 (A), c-MYC (B) and CYCLIN E (C) protein expression at the indicated CTs in s.c. tumors after repeated intra-tumoral DEX or PBS injection every 2 days for 8–11 days. Unstained control (red) and stained (blue) cells of the indicated antibody. (D) Representative flow cytometry dot plots for incorporated BrdU and staining with 7AAD at the indicated CTs in s.c. tumors after repeated intra-tumoral DEX or PBS injection every 2 days for 8–11 days. The illustrated gates indicate the analyzed cell cycle phases. Representative histogram for pHH3 (E) and histogram for Annexin V staining (F) at the indicated CTs in s.c. tumors after repeated intra-tumoral DEX or PBS injection every 2 days for 8–11 days. Positive (red) cells compared to unstained control cells (black). (PDF 2 MB)
Knockdown of Bmal1 prevents the DEX effects on B16 cell proliferation, cell cycle arrest and cell cycle phases. (A, B) Cell cycle arrest of Scrambled shRNA-transfected B16 cells (A) or Bmal1 shRNA-transfected B16 cells (B) indicated by cells in the G0 phase (left panels) and cell proliferation indicated by cells in the G1 phase (middle panels) or S/M/G2 phases (right panels) with control or DEX treatment (n = 5–6, wells/time point/group; two-way ANOVA, posthoc test, group effect: *p < 0.0.5, **p < 0.01, ***p < 0.001). (C–E) Cell cycle phases of Scrambled shRNA- and Bmal1 shRNA-transfected B16 cells after DEX treatment. Significant rhythms are illustrated with fitted cosine curves, otherwise data are connected by straight lines between data points, indicating no significant circadian rhythms (n = 10–15, 3–4 wells/time point; cosine-wave regression, F-test: p < 0.05; two-way ANOVA, posthoc test, group effect: **p < 0.01, ***p < 0.001). Frequencies of (F) B cells (CD19+), (G) dendritic cells (CD11c+), (H) CD4 T cells (CD4+), (I) CD8 T cells (CD8+), (J) macrophages (F4/80highLy6C-, gated on CD11b+), (K) neutrophils (F4/80 lowLy6Ghigh, gated on CD11b+) and (L) monocytes (CD11bhighLy6C+, gated on F4/80+) relative to alive cells after intra-tumoral PBS or DEX injection in B16 s.c. tumors of C57BL/6 J mice (Scrambled shRNA tumors and Bmal1 shRNA tumors: no significant difference between DEX and PBS throughout the experiment, n = 5–6 mice/group, Mann-Whitney rank sum test: p > 0.05). Data are represented as mean ± SEM. For details of statistics, see Additional file 1. (PDF 844 kb)
Immune cell infiltration, apoptosis and cell cycle arrest in NSG mice. Representative flow cytometry dot plots and quantification for neutrophils (F4/80 lowLy-6Ghigh, gated on CD11b+) (A), monocytes (CD11bhighLy-6Chigh, gated on F4/80+) (B), macrophages (F4/80highLy-6C- gated on CD11b+) (C), histogram and quantification for apoptosis (Annexin V) stained (red) and unstained (grey) cells (D) and dot plots and quantification of proliferation (Ki67) (E) at the indicated CTs in s.c. tumors after repeated intra-tumoral PBS or DEX injection every 2 days for 8–11 days in B16 s.c. tumors of NSG mice collected at CT14 (n = 4 mice/group, Mann-Whitney rank sum test: p > 0.05). (PDF 812 kb)
About this article
Cite this article
Kiessling, S., Beaulieu-Laroche, L., Blum, I.D. et al. Enhancing circadian clock function in cancer cells inhibits tumor growth. BMC Biol 15, 13 (2017). https://doi.org/10.1186/s12915-017-0349-7
- Circadian clock
- Clock gene expression
- Tumor growth
- Melanoma cancer
- Cell cycle checkpoints