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. 2018 Apr 10;18:126. doi: 10.1186/s12906-018-2192-y

Withania somnifera modulates cancer cachexia associated inflammatory cytokines and cell death in leukaemic THP-1 cells and peripheral blood mononuclear cells (PBMC’s)

Dhaneshree Bestinee Naidoo 1, Anil Amichund Chuturgoon 1, Alisa Phulukdaree 1, Kanive Parashiva Guruprasad 2, Kapaettu Satyamoorthy 2, Vikash Sewram 3,4,✉
PMCID: PMC5891897  PMID: 29631586

Abstract

Background

Cancer and inflammation are associated with cachexia. Withania somnifera (W. somnifera) possesses antioxidant and anti-inflammatory potential. We investigated the potential of an aqueous extract of the root of W. somnifera (WRE) to modulate cytokines, antioxidants and apoptosis in leukaemic THP-1 cells and peripheral blood mononuclear cells (PBMC’s).

Methods

Cytotoxcity of WRE was determined at 24 and 72 h (h). Oxidant scavenging activity of WRE was evaluated (2, 2-diphenyl-1 picrylhydrazyl assay). Glutathione (GSH) levels, caspase (− 8, − 9, − 3/7) activities and adenosine triphosphate (ATP) levels (Luminometry) were thereafter assayed. Tumour necrosis factor-α (TNF-α), interleukin (IL)-6, IL-1β and IL-10 levels were also assessed using enzyme-linked immunosorbant assay.

Results

At 24 h, WRE (0.2–0.4 mg/ml) decreased PBMC viability between 20 and 25%, whereas it increased THP-1 viability between 15 and 23% (p < 0.001). At 72 h, WRE increased PBMC viability by 27–39% (0.05, 0.4 mg/ml WRE) whereas decreased THP-1 viability between 9 and 16% (0.05–0.4 mg/ml WRE) (p < 0.001). Oxidant scavenging activity was increased by WRE (0.05–0.4 mg/ml, p < 0.0001). PBMC TNF-α and IL-10 levels were decreased by 0.2–0.4 mg/ml WRE, whereas IL-1β levels were increased by 0.05–0.4 mg/ml WRE (p < 0.0001). In THP-1 cells, WRE (0.05–0.4 mg/ml) decreased TNF-α, IL-1β and IL-6 levels (p < 0.0001). At 24 h, GSH levels were decreased in PBMC’s, whilst increased in THP-1 cells by 0.2–0.4 mg/ml WRE (p < 0.0001). At 72 h, WRE (0.1–0.4 mg/ml) decreased GSH levels in both cell lines (p < 0.0001). At 24 h, WRE (0.2–0.4 mg/ml) increased PBMC caspase (-8, -3/7) activities whereas WRE (0.05, 0.1, 0.4 mg/ml) increased THP-1 caspase (-9, -3/7) activities (p < 0.0001). At 72 h, PBMC caspase (-8, -9, -3/7) activities were increased at 0.05–0.1 mg/ml WRE (p < 0.0001). In THP-1 cells, caspase (-8, -9, -3/7) activities and ATP levels were increased by 0.1–0.2 mg/ml WRE, whereas decreased by 0.05 and 0.4 mg/ml WRE (72 h, p < 0.0001).

Conclusion

In PBMC’s and THP-1 cells, WRE proved to effectively modulate antioxidant activity, inflammatory cytokines and cell death. In THP-1 cells, WRE decreased pro-inflammatory cytokine levels, which may alleviate cancer cachexia and excessive leukaemic cell growth.

Electronic supplementary material

The online version of this article (10.1186/s12906-018-2192-y) contains supplementary material, which is available to authorized users.

Keywords: Cancer, Cachexia, Cytokines, Apoptosis, Withania somnifera

Background

Chronic inflammation plays an essential role in malignancies [1] through the initiation, promotion and progression of tumours [2]. Usually, the host-mediated anti-tumour activity overcomes the tumour-mediated immunosuppressive activity leading to the elimination of cancerous cells [2]. However, in the presence of an inadequate host anti-tumour defence, the pro-inflammatory tumour microenvironment is enhanced and promotes tumour development, invasion, angiogenesis and metastasis [2].

The cachectic syndrome is prominent in malignancies occurring in up to 50% of all cancer patients [3]. It is a progressive, debilitating condition leading to abnormal weight loss, as a result of adipose tissue (85%) and skeletal muscle (75%) depletion [3–5]. Modulation of lipogenesis and lipolysis is essential in maintaining adipose tissue mass. Lipoprotein lipase (LPL) hydrolyses fatty acids (FA’s) from plasma lipoproteins, thereafter FA’s are transported to adipose tissue for triacylglycerol (TAG) production, whereas hormone sensitive lipase (HSL) hydrolyses TAG’s into FA’s and glycerol [3]. Literature shows that decreased serum LPL levels/activity and increased HSL levels/activity are associated with cachexia [6–8]. Additionally, increased proteolysis [9] and decreased proteogenesis has been established in cachectic patients [10]. The ATP-ubiquitin-dependent proteolytic pathway has been shown to be responsible for the accelerated proteolysis seen in a variety of wasting conditions, including cancer cachexia [11].

Inflammatory cytokines, oxidative stress and apoptosis have been implicated in the initiation and progression of cancer, imbalance of catabolic/anabolic processes [12] and development of cachexia [13]. Production of inflammatory cytokines [tumour necrosis factor-α (TNF-α), interleukin (IL) – 6, and IL-1β] is activated by lipopolysaccharide (LPS) that potently stimulates macrophages [14, 15]. The LPS signal is transduced by LPS binding to LPS binding protein, delivered to CD14 and transferred to Toll like receptor-4 [16]. Nuclear factor kappa B (NF-κB) is subsequently activated and regulates the transcription of genes associated with inflammation, proliferation, invasion, angiogenesis and apoptosis [1, 17–19]. Pro-inflammatory cytokines (TNF-α, IL-6 and IL-1) have been shown to decrease LPL activity [20–23], which reduces the uptake of exogenous lipids by adipose tissue [21], ultimately decreasing lipogenesis. Additionally, previous studies have indicated that TNF-α increased ubiquitin (concentrations and mRNA), while IL-6 increased the 26S proteasome and cathepsins activities, which may activate proteolytic pathways [4, 24–26], ultimately increasing proteolysis. In combination, excessive levels of pro-inflammatory cytokines increase tumour suppressive activity [2] and tissue wasting [3].

Reactive oxygen species (ROS) have been associated with tumour initiation, inflammation [2, 27] and muscle wasting [28]. However, antioxidants have been shown to decrease muscle wasting by neutralizing ROS [1, 28]. Elevated ROS levels activate apoptotic pathways, ultimately activating caspase-3 [29]. Caspase-3 activation plays an essential role in the execution of apoptosis, as well as muscle proteolysis [30]. In addition, in weight losing upper gastro-intestinal tract cancer patients, deoxyribonucleic acid (DNA) fragmentation and poly (ADP-ribose) polymerase (PARP) cleavage were increased, whereas MyoD protein was decreased, indicating increased apoptosis and decreased muscle replenishment [3].

Cancer patients suffer from a wide range of side-effects caused by current cancer chemotherapeutic and radiotherapeutic agents. Patients are constantly seeking alternative traditional remedies to alleviate their discomfort. Withania somnifera (L.) Dunal (W. somnifera) is a well known medicinal plant cultivated in India, parts of East Asia and Africa [31]. It is commonly referred to as Ashwagandha and belongs to the Solanaceae family [31]. Compounds isolated from W. somnifera include withaferin A and 3-β-hydroxy-2, 3 dihydro withanolide F [32]. The major constituent of the root extract of W. somnifera is withanolide-A [33]. W. somnifera is frequently used in Ayurvedic medicine due to its various medicinal properties [31]. These properties include anti-inflammatory [34], antioxidant and immune-modulatory activities [35]. W. somnifera was found to be an immune regulator in inflammation animal models [36]. The immunosuppressive action of W. somnifera may be due to the presence of withanolides, steroidal lactones and a few flavanoids [37]. In addition, W. somnifera formulation (WSF) has shown anti-proliferative potential in human promyelocytic leukemia (HL-60) cells, by activating the intrinsic and extrinsic apoptotic pathways [38]. When used together, W. somnifera formulations aid the host to effectively fight cancer and reduce the harmful effects of chemotherapy and radiotherapy [39].

There is a need for the discovery of an inexpensive cancer cachectic treatment to improve the prognosis of cancer patients and to establish a mechanism of regulation of the immune system, inflammasome and apoptosis in order to prevent/decelerate the rapid depletion of skeletal muscle and adipose tissue. We investigated the effect of an aqueous extract of the root of W. somnifera (WRE) on antioxidant capacity, inflammatory cytokine levels and cell death induction in leukaemic THP-1 cells and peripheral blood mononuclear cells (PBMC’s).

Methods

Materials

The roots of W. somnifera were collected on the 11th of March 2011 (collectors number: Immelman 427) from the Eastern Cape [the Ntubeni Location near Dwesa Reserve], South Africa (SA) and identified by Dr. Kathleen Immelman from the Department of Botany at the Walter Sisulu University, SA and further comparison to South African data [40]. Voucher specimens were deposited at the KEI herbarium (13995). THP-1 cells were obtained from from American Type Culture Collection (ATCC, University Boulevard Manassas, Virginia, USA). RPMI-1640 and BD OptEIA enzyme-linked immunosorbant assay (ELISA) cytokine kits were purchased from The Scientific Group (Johannesburg, SA). Foetal calf serum (FCS) and Pen/Strep Amphotericin B (PSF) were acquired from Whitehead Scientific (Cape Town, SA). Dimethyl sulphoxide (DMSO) was purchased from Merck (Johannesburg, SA). Histopaque-1077, LPS and 2, 2-diphenyl-1 picrylhydrazyl (DPPH) were purchased from Sigma (Aston Manor, SA). The 4-[3-(4-iodophenyl)-2-(4-nitrophenyl)-2H-5-tetrazolio]-1,3-benzene disulphonate (WST-1) cell proliferation reagent was purchased from Roche (Johannesburg, SA). Promega (Madison, USA) supplied the caspase (-3/7, -8, -9), adenosine triphosphate (ATP) and glutathione (GSH) kits.

Plant extraction

The roots of W. somnifera were dried and milled before being sequentially extracted in ethanol and distilled water. Ethanol (200–350 ml) was added to the milled root (10–30 g) and extracted overnight by shaking (4×g, 37 °C). The ethanol extracts were thereafter filtered, evaporated using a rotary evaporator, dried (37 °C) and stored (4 °C). The root material was thereafter extracted with distilled water (200–350 ml) by shaking (4×g, 75 °C) for a period of 6 hours (h). Water extracts were filtered, dried and stored (4 °C).

The 2, 2-diphenyl-1 picrylhydrazyl assay

WRE (0.05–0.4 mg/ml) and butylated hydroxytoluene (BHT) (60–300 μM) dilutions were prepared in methanol (99.5% and grade AR). A 50 μM DPPH solution was prepared from a stock solution of 0.135 mM DPPH in methanol. WRE, BHT dilutions and methanol (1 ml) were aliquoted into 15 ml polypropylene tubes, followed by the 50 μM DPPH solution (1 ml). Reaction mixtures were vortexed and incubated [room temperature (RT), 30 min (min)] in the dark. Absorbance of samples was read at 517 nm using a Varine Cary 50 UV-visible spectrophotometer (McKinley Scientific, New Jersey, US).

Isolation of peripheral blood mononuclear cells

Buffy coats containing PBMC’s were obtained from the South African National Blood Service (2011/09). PBMC’s were extracted by differential centrifugation. Buffy coats (5 ml) were layered onto equivolume histopaque-1077 (5 ml) in 15 ml polypropylene tubes and centrifuged (400×g, 21 °C for 30 min). After centrifugation, the PBMC’s were transferred to sterile 15 ml polypropylene tubes, phosphate buffered saline (PBS) was added (0.1 M, 10 ml) and tubes were centrifuged (400×g, 21 °C, 15 min). Cell density of isolated PBMC’s was adjusted (1 × 106 cells/ml) using the trypan blue exclusion test and cryo-preserved (10% FCS, 10% DMSO) using a NELGENE cryo freezing container and stored at -80 °C.

Tissue culture

THP-1 cells were grown in the appropriate tissue culture conditions in a 75 cm3 tissue culture flask (37 °C, 5% CO2). The growth media comprised of RPMI-1640, FCS (10%) and PSF (2%). Cells were thawed, seeded into a 75 cm3 tissue culture flask at a concentration of 3 × 105 cells/ml and incubated (37 °C, 5% CO2). THP-1 cells were allowed to grow for 2–3 days before the cells were centrifuged (162×g, 10 min) and re-suspended in fresh growth media. The number of cells should not exceed 8 × 105 cells/ml, therefore the cells/ml was quantified daily by trypan blue staining. Once the cell count reached 8 × 105 cells/ml the THP-1 cells were split/diluted to 3 × 105 cells/ml with media and incubated. Subsequent experiments were conducted once the cell numbers were sufficient.

Cell viability assay

Cytotoxicity of WRE in PBMC’s and THP-1 cells was measured using the WST-1 assay (Roche, Johannesburg, SA). PBMC and THP-1 cells (10,000 cells/well, 96-well plate, in triplicate wells) were stimulated with LPS (20 μg/ml, 37 °C, 5% CO2, 4 h) before exposure to WRE (0.05–0.4 mg/ml) for 24 and 72 h (37 °C, 5% CO2). Similarly, controls received media. Thereafter, plates were centrifuged (162×g, 10 min), supernatant removed, cell pellets re-suspended in growth media (100 μl/well), WST-1 reagent (10 μl/well) added and plates incubated (37 °C, 5%, CO2, 3 h). Optical density was measured at 450 nm (620 nm reference wavelength) with a BIO-TEK μQuant spectrophotometer (Analytical and Diagnostic Products, SA). This experiment was conducted independently on three occasions.

Stimulation and treatment of cells

PBMC’s and THP-1 cells (1 × 105 cells/ml) were transferred into 24-well plates and stimulated with LPS (20 μg/ml, 37 °C, 5% CO2, 4 h) before exposure to WRE (0.05–0.4 mg/ml) for 24 h (TNF-α) and 72 h (IL-1β, IL-6, IL-10) (37 °C, 5% CO2). After incubation, plates were centrifuged (162×g, 10 min) and the supernatant collected and stored (− 80 °C) for cytokine analysis. Cell pellets were used to conduct the caspase (-8, -9, -3/7) activity, as well as ATP and GSH assays. The experiments were conducted independently (twice) for all subsequent assays.

Quantification of cytokines

Cytokine levels were estimated using the BD OptEIA ELISA kits (The Scientific Group, SA) and the procedure was followed as per the instruction manual. ELISA plates were coated with capture antibody overnight (100 μl/well, 4 °C). Thereafter, plates were washed (3×) with wash buffer and blocked with assay diluent (200 μl/well, 1 h, RT). Standard solutions were prepared by diluting a stock solution [TNF-α, IL-10 (500 pg/ml), IL-6 (300 pg/ml), IL-1β (250 pg/ml)] serially [TNF-α, IL-10 (500–7.8 pg/ml), IL-6 (300–4.7 pg/ml), IL-1β (250–3.9 pg/ml)]. Plates were washed (3×), standards and samples (100 μl/well) were aliquoted into appropriate wells and plates were incubated (2 h, RT). Plates were washed (5×), working detector (100 μl/well) added and plates incubated (1 h, RT). The plates were washed (7×), substrate solution (100 μl/well) added and plates were incubated (30 min, RT) in the dark. Finally, stop solution (50 μl/well) was added and the absorbance was read at 450 nm (570 nm reference wavelength) with a Multiskan FC micro-plate reader (Thermo Scientific). Cytokine concentrations were calculated by extrapolation from a standard curve.

The glutathione assay

The GSH-Glo™ assay (Promega, Madison, USA) was performed to measure GSH levels. Standard GSH solutions were prepared by diluting a 5 mM stock solution serially (1.56–50 μM) and PBS (0.1 M) was the standard blank. Cells (50 μl/well, 2 × 105 cells/ml) and standards were added into an opaque 96-well plate, followed by GSH-Glo™ reagent (25 μl/well) and allowed to incubate (30 min, RT) in the dark. Luciferin detection reagent (50 μl/well) was subsequently added and plates incubated (15 min, RT) in the dark. The absorbance was read on a Modulus™ microplate luminometer (Turner Biosystems, Sunnyvale, USA) and GSH concentrations were calculated by extrapolation from a standard curve.

Caspase and ATP assays

Caspase activity and ATP levels were determined using the Caspase-Glo®-3/7, -8, -9 and ATP assay kits (Promega, Madison, USA). Caspase-Glo®-3/7, -8, -9 and ATP reagents were reconstituted according to the manufacturer’s instructions. Cells (100 μl, 2 × 105 cells/ml) were added into duplicate wells of a microtitre plate for each assay, thereafter caspase -3/7, -8, -9 and ATP reagents (100 μl/well) were added into appropriate wells. The plate was incubated (30 min, RT) in the dark. Luminescence was measured on a Modulus™ microplate luminometer (Turner BioSystems) and expressed as relative light units (RLU).

Statistical analysis

Statistical analysis was performed using the STATA and GraphPad Prism statistical analysis software. The one-way analysis of variance (ANOVA) was used to compare between groups, followed by the Tukey multiple comparisons test, with p < 0.05 defining statistical significance.

Results

The oxidant scavenging potential of WRE

The oxidant scavenging activity of WRE using the DPPH assay is shown in Fig. 1. WRE (0.05–0.4 mg/ml) significantly increased DPPH scavenging activity by 13.33–46.38% (Fig. 1, p < 0.0001).

Fig. 1.

Fig. 1

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Percentage DPPH scavenging activity of WRE (Values expressed as mean ± SD, * p < 0.05, *** p < 0.0001, compared to control)

The in vitro cytotoxicity of WRE

The WST-1 assay was used to determine cell viability of THP-1 cells and PBMC’s after treatment with WRE (Fig. 2). At 24 h, WRE (0.05–0.4 mg/ml) decreased PBMC viability by 20.69–25.15% while WRE (0.2–0.4 mg/ml) increased THP-1 viability by 15.99–22.54% as compared to the controls (Fig. 2a and c, p < 0.001). This result suggests that PBMC’s are more sensitive to WRE treatment than THP-1 cells.

Fig. 2.

Fig. 2

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Cell viability of PBMC’s (a – 24 h, b – 72 h) and THP-1 (c – 24 h, d – 72 h) cells treated with WRE for 24 and 72 h (Values expressed as mean ± SD, * p < 0.05,** p < 0.005, *** p < 0.0001 compared to the control)

At 72 h, PBMC viability was increased (27.16–38.58%) by WRE (0.05, 0.4 mg/ml), as compared to the control (Fig. 2b, p < 0.0001). In the same time period, WRE (0.05–0.4 mg/ml) decreased THP-1 viability by 9.07–16.09% relative to the control (Fig. 2d, p=0.0002).

The immune suppressive properties of WRE

WRE altered cytokine levels in PBMC’s and THP-1 cells (Fig. 3 and Fig. 4). The levels of TNF-α, IL-1β, IL-6 and IL-10 produced by LPS stimulated PBMC’s was 336.218, 168.100, 657.878 and 46.990 pg/ml respectively. WRE (0.2–0.4 mg/ml) decreased PBMC TNF-α and IL-10 levels as compared to the control (Fig. 3a and d, p < 0.0001). In PBMC’s, IL-6 levels were decreased by 0.4 mg/ml WRE, whereas IL-1β levels were increased by 0.05–0.4 mg/ml WRE relative to the control (Fig. 3b and c, p < 0.0001).

Fig. 3.

Fig. 3

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Concentration of TNF-α (a), IL-1β (b), IL-6 (c) and IL-10 (d) in LPS stimulated and WRE treated PBMC’s (Values expressed as mean ± SD, *p < 0.05, *** p < 0.0001, compared to the control)

Fig. 4.

Fig. 4

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Concentration of TNF-α (a), IL-1β (b), IL-6 (c) and IL-10 (d) in LPS stimulated and WRE treated THP-1 cells (Values expressed as mean ± SD, *p < 0.05, ***p < 0.0001 compared to the control)

The levels of TNF-α, IL-1β, IL-6 and IL-10 produced by LPS stimulated THP-1 cells were 13.285, 21.947, 78.622 and 2.705 pg/ml respectively. In THP-1 cells, TNF-α, IL-1β and IL-6 levels were decreased by 0.05–0.4 mg/ml WRE, whilst IL-10 levels were decreased by 0.4 mg/ml WRE as compared to the control (Fig. 4, p < 0.003).

The antioxidant potential of WRE

The endogenous antioxidant activity of WRE was determined by measuring GSH levels in both cell lines (Table 1). At 24 h, GSH levels in PBMC’s were decreased by WRE (0.05, 0.2, 0.4 mg/ml) relative to the control (Table 1, p < 0.0001). In THP-1 cells, GSH levels were decreased at 0.05 mg/ml WRE whereas increased (0.41–1.62 μM) at 0.1–0.4 mg/ml WRE compared to the control (Tables 1, 24 h, p < 0.0001).

Table 1.

Glutathione levels in LPS stimulated and WRE treated PBMC’s and THP-1 cells

Glutathione (μM)
WRE (mg/ml) 24 h Treatment 72 h Treatment
PBMC THP-1 PBMC THP-1
Control 1.613 ± 0.017 1.632 ± 0.004 4.799 ± 0.008 1.608 ± 0.004
0.05 1.442 ± 0.024 *** 1.267 ± 0.004 *** 5.232 ± 0.011 *** 1.548 ± 0.002 ***
0.1 1.617 ± 0.002 2.045 ± 0.002 *** 4.015 ± 0.001 *** 1.589 ± 0.004 ***
0.2 1.390 ± 0.001 *** 3.253 ± 0.017 *** 2.323 ± 0.005 *** 1.401 ± 0.006 ***
0.4 1.321 ± 0.006 *** 2.785 ± 0.005 *** 4.697 ± 0.003 *** 1.411 ± 0.005 ***
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(Values expressed as mean ± SD, *** p < 0.0001, compared to the control)

At 72 h, PBMC GSH levels were increased at 0.05 mg/ml whereas decreased 0.1–0.4 mg/ml WRE compared to the control (Table 1, p < 0.0001). WRE (0.05–0.4 mg/ml) decreased GSH levels in THP-1 cells relative to the control (Tables 1, 72 h p < 0.0001).

WRE modulates caspase (-8, -9, -3/7) activities and ATP levels

Luminometry assays were used to determine caspase activity and ATP levels in THP-1 cells and PBMC’s after treatment with WRE. The pro-apoptotic effect of WRE in PBMC’s treated for 24 h is shown in Table 2. At 24 h, PBMC caspase-8 activity was decreased by 0.05 mg/ml WRE whereas increased by 0.2–0.4 mg/ml WRE compared to the control (Table 2, p < 0.0001). PBMC caspase-9 activity was increased by 0.05 and 0.2 mg/ml WRE but decreased by 0.1 and 0.4 mg/ml WRE relative to the control (Table 2, p < 0.0001). In PBMC’s, the increased caspase activity may be related to the decreased GSH levels at 24 h. A decrease in GSH levels may allow for an increase in ROS levels which can activate apoptotic pathways. Caspase-3/7 activity was increased in PBMC’s by 0.05–0.4 mg/ml WRE compared to the control (Table 2, p < 0.0001), suggesting an increased execution of apoptotic cell death. In azoxymethane-induced colon cancer in mice, W. somnifera has been shown to modulate TCA cycle enzymes and the electron transport chain [41]. The PBMC ATP levels were increased by 0.1, 0.4 mg/ml WRE but decreased by 0.05, 0.2 mg/ml WRE compared to the control (Table 2, p < 0.0001), which may be related to the modulation of the electron transport chain by W. somnifera.

Table 2.

Modulation of caspase (-8, -9, -3/7) activity and ATP levels in LPS stimulated and 24 h WRE treated PBMC’s

WRE (mg/ml) Caspase-8 (RLU ×  105) Caspase-9 (RLU ×  105) Caspase-3/7 (RLU ×  105) ATP (RLU ×  105)
Control 0.185 ± 0.006 0.366 ± 0.0003 7.756 ± 0.006 4.714 ± 0.004
0.05 0.155 ± 0.0002 *** 0.376 ± 0.001 *** 8.109 ± 0.094 ** 2.783 ± 0.017 ***
0.1 0.192 ± 0.00002 0.253 ± 0.0002 *** 11.504 ± 0.253 *** 5.208 ± 0.005 ***
0.2 0.246 ± 0.0003 *** 0.397 ± 0.0005 *** 8.961 ± 0.015 *** 3.741 ± 0.033 ***
0.4 4.814 ± 0.006 *** 0.351 ± 0.001 *** 17.095 ± 0.089 *** 6.965 ± 0.039 ***
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(Values expressed as mean ± SD, ** p < 0.005, *** p < 0.0001 compared to the control)

WRE pro-apoptotic effects in THP-1 cells treated for 24 h are shown in Table 3. At 24 h, THP-1 caspase-9 activity was decreased by 0.2 mg/ml WRE but increased by 0.05, 0.1, 0.4 mg/ml WRE compared to the control (Table 3, p < 0.0001). At 0.2 mg/ml WRE, the decreased caspase-9 activity may be related to the increased GSH levels. An increase in GSH levels may decrease ROS levels thus minimising mitochondrial depolarisation and the activation of the intrinsic apoptotic pathway. In THP-1 cells, WRE (0.05–0.4 mg/ml) decreased caspase-8 activity, whereas increased caspase-3/7 activity and ATP levels relative to the control (Table 3, p < 0.0001). Elevated caspase (-9, -3/7) activities suggests the initiation of the mitochondrial apoptotic pathway.

Table 3.

Modulation of caspase (-8, -9, -3/7) activity and ATP levels in LPS stimulated and 24 h WRE treated THP-1 cells

WRE (mg/ml) Caspase-8 (RLU ×  105) Caspase-9 (RLU ×  105) Caspase-3/7 (RLU ×  105) ATP (RLU ×  105)
Control 10.207 ± 0.011 1.040 ± 0.007 1.251 ± 0.016 2.636 ± 0.011
0.05 8.440 ± 0.039 *** 2.365 ± 0.005 *** 1.315 ± 0.005 *** 3.726 ± 0.005 ***
0.1 2.413 ± 0.005 *** 2.459 ± 0.002 *** 2.294 ± 0.006 *** 5.132 ± 0.014 ***
0.2 7.149 ± 0.027 *** 0.775 ± 0.002 *** 3.406 ± 0.006 *** 29.838 ± 0.186 ***
0.4 2.456 ± 0.033 *** 3.197 ± 0.0001 *** 9.428 ± 0.004 *** 10.282 ± 0.195 ***
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(Values expressed as mean ± SD, *** p < 0.0001 compared to the control)

The pro-apoptotic effect of WRE in PBMC’s treated for 72 h is shown in Table 4. At 72 h, PBMC caspase-8 activity was increased by 0.05–0.2 mg/ml WRE but decreased by 0.4 mg/ml WRE compared to the control (Table 4, p < 0.0001). PBMC caspase-9 activity was increased by 0.05–0.1 mg/ml WRE but decreased by 0.2–0.4 mg/ml WRE relative to the control (Table 4, p < 0.0001). In PBMC’s, caspase-3/7 activity was increased by 0.05, 0.1, 0.4 mg/ml WRE whereas it decreased by 0.2 mg/ml WRE compared to the control (Table 4, p < 0.0001). At 0.05–0.1 mg/ml WRE, the increased caspase-3/7 activity is consistent with the significantly increased caspase -8 and -9 activity. At 0.2 mg/ml WRE, caspase-8 activity was minimally increased and caspase-9 activity significantly decreased which lead to the decreased caspase-3/7 activity. At 0.4 mg/ml WRE, although both caspase -8 and -9 activities were decreased, caspase-3/7 activity was increased. A previous study has demonstrated that one activated executioner caspase can cleave and activate other executioner caspases resulting in positive feedback loop of caspase activation [42] which may account for the increased caspase-3/7 activity at 0.4 mg/ml WRE. WRE (0.05–0.4 mg/ml) decreased PBMC ATP levels relative to the control (Table 4, p < 0.0001).

Table 4.

Modulation of caspase (-8, -9, -3/7) activity and ATP levels in LPS stimulated and 72 h WRE treated PBMC’s

WRE (mg/ml) Caspase-8 (RLU ×  105) Caspase-9 (RLU ×  105) Caspase-3/7 (RLU ×  105) ATP (RLU ×  105)
Control 42.651 ± 0.039 115.041 ± 3.848 155.556 ± 0.387 20.574 ± 0.316
0.05 53.840 ± 0.026 *** 143.861 ± 3.929 *** 196.471 ± 0.338 *** 10.223 ± 0.046 ***
0.1 52.109 ± 0.009 *** 129.033 ± 0.289 *** 192.695 ± 0.233 *** 12.506 ± 0.373 ***
0.2 42.751 ± 0.039 ** 105.494 ± 4.247 ** 154.203 ± 0.224 *** 13.210 ± 0.043 ***
0.4 29.656 ± 0.007 *** 92.718 ± 0.021 *** 165.139 ± 0.096 *** 13.361 ± 0.279 ***
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(Values expressed as mean ± SD,** p < 0.005, *** p < 0.0001 compared to the control)

WRE pro-apoptotic effects in THP-1 cells treated for 72 h are shown in Table 5. At 72 h, THP-1 caspase (-8, -9, -3/7) activity and ATP levels were increased by 0.1–0.2 mg/ml WRE as compared to the control (Table 5, p < 0.0001), suggesting an increase in THP-1 apoptotic cell death. THP-1 caspase (-8, -9, -3/7) activity and ATP levels were decreased by 0.05, 0.4 mg/ml WRE relative to the control (Table 5, 72 h, p < 0.0001), suggesting a decrease in THP-1 apoptosis.

Table 5.

Modulation of caspase (-8, -9, -3/7) activity and ATP levels in LPS-stimulated and 72 h WRE-treated THP-1 cells

WRE (mg/ml) Caspase-8 (RLU ×  105) Caspase-9 (RLU ×  105) Caspase-3/7 (RLU ×  105) ATP (RLU ×  105)
Control 0.991 ± 0.0001 5.738 ± 0.002 7.463 ± 0.012 4.332 ± 0.002
0.05 0.978 ± 0.0001 *** 5.562 ± 0.009 *** 6.919 ± 0.003 *** 4.133 ± 0.005 ***
0.1 1.216 ± 0.001 *** 7.045 ± 0.005 *** 8.211 ± 0.002 *** 4.889 ± 0.005 ***
0.2 1.095 ± 0.001 *** 6.091 ± 0.001 *** 7.532 ± 0.006 *** 4.576 ± 0.004 ***
0.4 0.952 ± 0.0003 *** 5.639 ± 0.003 *** 6.626 ± 0.007 *** 4.039 ± 0.0003 ***
Open in a new tab

(Values expressed as mean ± SD, *** p < 0.0001 compared to the control)

Discussion

Cachexia patients experience excessive weight loss due to increased lipolysis and proteolysis which have been linked to elevated levels of pro-inflammatory cytokines, oxidative stress and apoptosis [3, 5, 30]. Previously, the powdered root of W. somnifera displayed immune modulatory properties [43] and WSF has been shown to increase caspase-3 activity, subsequently inducing apoptosis [38]. The objective of this study was thus to investigate the modulation of cytokines, antioxidants and cell death by WRE in PBMC’s and THP-1 cells.

Dhanani et al. (2017) showed that the root extract of W. somnifera inhibited 50% of DPPH at a concentration of 0.4 mg/ml [44]. Our results indicated that WRE has oxidant scavenging potential ranging between 13 and 46% at 0.05–0.4 mg/ml. ROS plays an essential role in tumour initiation, inflammation, protein degradation and apoptosis. The antioxidant potential of WRE may decrease inflammatory cytokine levels as well as ROS induced apoptosis.

At 24 h, the WST-1 results indicated that WRE decreased PBMC viability whilst increasing THP-1 viability. However at 72 h, WRE increased PBMC viability whilst conversely decreasing THP-1 viability. In contrast, the growth of various cell lines (HT-29, HCT-15, SW620, 502,713, Colo-205, A549, HOP-62 and Hep-G2) were dose dependently inhibited by WSF and 50% cell growth inhibition was seen at 30 μg/ml WSF [38].

The pivotal role of inflammatory cytokines in malignancies and cachexia has been extensively documented [3]. Dhuley (1997) previously reported that W. somnifera inhibits macrophage production of inflammatory cytokines (IL-1, TNF-α) [45]. Our results showed that WRE decreased PBMC TNF-α, IL-10 and IL-6 levels, although it increased IL-1β levels. In THP-1 cells, pro-inflammatory cytokine (TNF-α, IL-1β, IL-6) levels were significantly decreased by WRE.

Pro-inflammatory cytokines, over a longstanding time period, stimulate the production of genotoxic molecules [nitric oxide (NO), ROS] and tumour progression by promoting angiogenesis and metastasis [1, 2]. In addition, pro-inflammatory cytokines activate NF-κB which regulates the expression of genes involved in the suppression of tumour apoptosis, stimulation of tumour cell cycle progression and enhancement of inflammatory mediators [1, 2]. NF-κB promotes tumour progression, invasion, angiogenesis and metastasis [1, 2].

Previous literature has shown that IL-1 stimulates growth and invasion of malignant cells [2]. Additionally, IL-6 has been shown to target cell cycle progression and anti-apoptotic genes leading to tumour proliferation and anti-apoptotic potential [2]. The ability of WRE to increase pro-inflammatory cytokines such as IL-1β in PBMC’s may aid in cancerous cell elimination through increased host anti-tumour activity. Conversely, in THP-1 cells, the decrease in TNF-α, IL-6 and IL-1β levels by WRE may prevent excessive activation of NF-κB, diminish cytokine induced tumour immunosuppressive activity and cancer progression.

With regard to cancer cachexia, IL-6 decreased LPL activity in adipose tissue of mice [22] and IL-1 directly modulates lipid metabolism by suppressing LPL activity [23]. TNF-α decreased LPL activity in adipose tissue of human (maintained in organ culture), rat, mouse, and guinea pigs [21]. Additionally, TNF-α inhibits the production of LPL and reduces the rate of LPL gene transcription in mouse 3 T3-L1 adipocytes, hence preventing the formation of new lipid stores while stimulating HSL and increasing lipolysis [3, 20, 46]. The potential of WRE to decrease pro-inflammatory cytokine levels in PBMC’s and THP-1 cells suggests a decrease in LPL inhibition and HSL stimulation, thus maintaining lipogenesis and minimizing lipolysis. IL-6 and TNF-α further contribute to cachexia by stimulating muscle catabolism via the activation of proteasome pathways [24, 25, 47]. In cachexia, NF-κB activation induces ubiquitin–proteasome pathway activity and suppresses MyoD expression [48], thereby increasing proteolysis and reducing muscle replenishment [49]. By decreasing TNF-α and IL-6 levels in PBMC’s and THP-1 cells, WRE may prevent excessive activation of NF-κB and proteasome pathways, ultimately decreasing proteolysis associated with the cachectic syndrome. Taken together, WRE may be able to decrease tissue wasting through the down regulation of pro-inflammatory cytokine levels.

The immunosuppressive and anti-inflammatory cytokine, IL-10, inhibits tumour development, tumour progression, modulates apoptosis and suppresses angiogenesis during tumour regression [1, 2]. Additionally, IL-10 inhibits NF-κB activation and subsequently inhibits pro-inflammatory cytokine production (TNF-α, and IL-6) [2]. In PBMC’s and THP-1 cells, the decreased IL-10 levels may be due to IL-10 combating increased pro-inflammatory cytokines levels (TNF-α, IL-6, IL-1β).

Antioxidants protect cells from increased oxidative stress [50]. GSH is a potent antioxidant that effectively scavenges ROS both directly and indirectly [50]. W. somnifera has previously been shown to possess chemo-preventive activity which may be a consequence of its antioxidant capacity [39]. The 24 h results showed that WRE decreased GSH levels in PBMC’s, whereas it increased GSH levels in THP-1 cells. However, at 72 h, WRE decreased GSH levels in both cell lines. Notably, GSH levels (72 h) were higher in control PBMC’s (4.79 μM) compared to control THP-1 cells (1.61 μM), suggesting a higher oxidant defence in PBMC’s.

The extrinsic (death receptors) and intrinsic (mitochondria) pathways are the two main apoptotic pathways [29]. Activation of initiator caspases (-8, -9) leads to the activation of executioner caspases (-3/7) resulting in activation of cytoplasmic endonucleases [29]. In HL-60 cells, WSF treatment led to a loss of mitochondrial membrane potential, translocation of Bax to mitochondria, release of cytochrome c, Smac/DIABLO and apoptosis inducing factor, suggesting the activation of the intrinsic apoptotic pathway [38]. Additionally, WSF treated HL-60 cells showed an over-expression of TNF receptor-1 and death receptor-4 with associated caspase-8 activation, suggesting the activation of the extrinsic apoptotic pathway [38]. Our 24 h results showed that WRE increased PBMC caspase -8, -9 and -3/7 activities at different concentrations, suggesting the activation of extrinsic and intrinsic apoptotic pathways. In the same time period, WRE increased THP-1 caspase -9 and -3/7 activities, suggesting initiation of apoptosis through the intrinsic pathway. At 72 h, WRE (0.05–0.1 mg/ml) increased caspase (-8, -9, -3/7) activities, suggesting an increased initiation of PBMC apoptotic cell death. However, 0.4 mg/ml WRE decreased initiator caspase (-8, -9) activities, suggesting a decreased initiation of PBMC apoptotic cell death. In THP-1 cells, 0.1–0.2 mg/ml WRE (72 h) increased caspase (-8, -9, -3/7) activities, suggesting initiation of apoptosis through the intrinsic and extrinsic pathways. However, at 0.05 and 0.4 mg/ml WRE (72 h), THP-1 caspase (-8, -9, -3/7) activities were decreased, suggesting a decrease in THP-1 apoptosis. Previous studies have indicated that W. somnifera may activate the extrinsic and intrinsic apoptotic pathways [38], therefore our results prove to be consistent with other studies.

Increased caspase-3 activity, proteasome activity and E3 ubiquitin-conjugating enzyme expression is associated with increased proteolysis [51]. Therefore the ability of WRE (0.4 mg/ml, 72 h) to down regulate caspase activity in PBMC’s and THP-1 cells may decrease proteolysis and the progression of cancer cachexia.

A successful anti-cancer drug should kill or incapacitate cancer cells without causing excessive damage to normal cells [39]. The potential of WRE to regulate PBMC apoptosis while increasing cancerous THP-1 cell apoptosis may be beneficial to cancer patients by preventing excessive cancerous cell growth while minimally effecting healthy PBMC’s.

Conclusion

The cachectic syndrome decreases the quality of life of patients, the responsiveness to chemotherapy and leads to 20–25% of cancer deaths [3]. Our results show that WRE increased oxidant scavenging activity, modulated GSH and pro-inflammatory cytokine levels and regulated caspase activity in normal PBMC’s and THP-1 cells. The discovery of a medicinal plant capable of decreasing the levels of pro-inflammatory cytokines may decrease tissue wasting. In this study, the root extract of W. somnifera has shown promising results in modulating the production of cytokines associated with cancer cachexia. The ability of WRE to decrease pro-inflammatory cytokine levels and increase cancerous cell death may decrease the development and progression of cancer and cachexia. WRE may therefore be effective in cancer cachexia.

Additional file

Additional file 1: (288.9KB, xlsx)

Assay data from root extract of W. Somnifera. (XLSX 288 kb)

Acknowledgements

We are grateful to the National Research Foundation, the South African Medical Research Council, Department of Science and Technology, Government of India and Manipal University for financial support to conduct experimentation. The authors also acknowledge Miss Tarylee Reddy for assistance with statistical analysis of data.

Funding

Sources of funding included the National Research Foundation, the South African Medical Research Council and Department of Science and Technology, Government of India and Manipal University, India. The funding sources were not involved in study design, collection of samples, analysis of data, interpretation of data, writing of the report and decision to publish. Scientific output is a requirement of the National Research Foundation.

Availability of data and materials

All data generated or analysed during this study are included in this published article as a Additional file 1.

Abbreviations

ATP

Adenosine triphosphate

BHT

butylated hydroxytoluene

DNA

Deoxyribonucleic acid

DPPH

2, 2-diphenyl-1 picrylhydrazyl

ELISA

enzyme-linked immunosorbant assay

FA’s

fatty acids

FCS

Foetal calf serum

GSH

Gluthatione

h

Hours

HL-60

Human promyelocytic leukemia

HSL

hormone sensitive lipase

IL

interleukin

LPL

lipoprotein lipase

LPS

lipopolysaccharide

min

Minute

NF-κB

Nuclear factor kappa B

NO

nitric oxide

PARP

poly (ADP-ribose) polymerase

PBMC’s

peripheral blood mononuclear cells

PBS

phosphate buffered saline

PSF

Pen/Strep Amphotericin B

RLU

Relative light units

ROS

reactive oxygen species

RT

room temperature

SA

South Africa

TAG

triacylglycerol

THP-1

leukemic cell line

TNF-α

tumour necrosis factor-α

W. somnifera

Withania somnifera

WRE

W. somnifera aqueous root extract

WSF

W. somnifera formulation

WST-1

4-[3-(4-iodophenyl)-2-(4-nitrophenyl)-2H-5-tetrazolio]-1,3-benzene disulfonate

Authors’ contributions

DBN carried out all experimentation except the luminometry (Caspase, ATP, GSH) assays. DBN analysed and interpreted data, performed statistical analysis, drafted and revised the manuscript. AC and AP carried out luminometry assays and provided intellectual input into the manuscript. VS, KPG and KS gave substantial contributions to conception, design and supervision of the study and revision of the manuscript. All authors read and approved the final manuscript.

Ethics approval and consent to participate

Collection of PBMC’s was approved by the Ethics Committee of the South African Medical Research Council (EC09–018) and the South African National Blood Service (2011/09).

Consent for publication

Not applicable.

Competing interests

The author(s) declare that they have no competing interests.

Publisher’s Note

Springer Nature remains neutral with regard to jurisdictional claims in published maps and institutional affiliations.

Footnotes

Electronic supplementary material

The online version of this article (10.1186/s12906-018-2192-y) contains supplementary material, which is available to authorized users.

Contributor Information

Dhaneshree Bestinee Naidoo, Email: bestinee@gmail.com.

Anil Amichund Chuturgoon, Email: CHUTUR@ukzn.ac.za.

Alisa Phulukdaree, Email: alisa.phulukdaree@up.ac.za.

Kanive Parashiva Guruprasad, Email: guruprasad.kp@manipal.edu.

Kapaettu Satyamoorthy, Email: ksatyamoorthy@manipal.edu.

Vikash Sewram, Phone: 27-21-927-7001, Email: vsewram@sun.ac.za.

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Associated Data

This section collects any data citations, data availability statements, or supplementary materials included in this article.

Supplementary Materials

Additional file 1: (288.9KB, xlsx)

Assay data from root extract of W. Somnifera. (XLSX 288 kb)

Data Availability Statement

All data generated or analysed during this study are included in this published article as a Additional file 1.

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