- About this Journal ·
- Abstracting and Indexing ·
- Advance Access ·
- Aims and Scope ·
- Annual Issues ·
- Article Processing Charges ·
- Articles in Press ·
- Author Guidelines ·
- Bibliographic Information ·
- Citations to this Journal ·
- Contact Information ·
- Editorial Board ·
- Editorial Workflow ·
- Free eTOC Alerts ·
- Publication Ethics ·
- Reviewers Acknowledgment ·
- Submit a Manuscript ·
- Subscription Information ·
- Table of Contents
Evidence-Based Complementary and Alternative Medicine
Volume 2012 (2012), Article ID 701927, 11 pages
Fractionation of an Extract of Pluchea odorata Separates a Property Indicative for the Induction of Cell Plasticity from One That Inhibits a Neoplastic Phenotype
1Institute of Clinical Pathology, Medical University of Vienna, Waehringer Guertel 18-20, 1090 Vienna, Austria
2Department of Pharmacognosy, Faculty of Life Sciences, University of Vienna, AlthanstraBe 14, 1090 Vienna, Austria
3Department of Nutritional Sciences, Faculty of Life Sciences, University of Vienna, AlthanstraBe 14, 1090 Vienna, Austria
4Clinical Institute of Medical and Chemical Laboratory Diagnostics, Medical University of Vienna, Waehringer Guertel 18-20, 1090 Vienna, Austria
5Institute for Ethnobiology, Playa Diana, San José, Petén, Guatemala
6Finzelberg GmbH & Co. KG, Koblenzer Strasse 48-54, 56626 Andernach, Germany
Received 29 September 2011; Accepted 6 December 2011
Academic Editor: Ashok D. Taranalli
Copyright © 2012 Mareike Seelinger et al. This is an open access article distributed under the Creative Commons Attribution License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original work is properly cited.
Introduction. Several studies demonstrated that anti-inflammatory remedies exhibit excellent anti-neoplastic properties. An extract of Pluchea odorata (Asteraceae), which is used for wound healing and against inflammatory conditions, was fractionated and properties correlating to anti-neoplastic and wound healing effects were separated. Methods. Up to six fractionation steps using silica gel, Sephadex columns, and distinct solvent systems were used, and eluted fractions were analysed by thin layer chromatography, apoptosis, and proliferation assays. The expression of oncogenes and proteins regulating cell migration was investigated by immunoblotting after treating HL60 cells with the most active fractions. Results. Sequential fractionations enriched anti-neoplastic activities which suppressed oncogene expression of JunB, c-Jun, c-Myc, and Stat3. Furthermore, a fraction (F4.6.3) inducing or keeping up expression of the mobility markers MYPT, ROCK1, and paxillin could be separated from another fraction (F4.3.7), which inhibited these markers. Conclusions. Wound healing builds up scar or specific tissue, and hence, compounds enhancing cell migration support this process. In contrast, successful anti-neoplastic therapy combats tumour progression, and thus, suppression of cell migration is mandatory.
Drug discovery is a constant need for biomedical research and clinical progress. Particularly mega-biodiversity areas such as the tropical rainforests of Central America are very promising for the discovery of new pharmaceutical lead compounds. Therefore, we chose an ethnomedical approach to drug discovery and focussed on traditional remedies of the Maya to preselect plants with proven health effects.
Traditional medicine plants are often used for hundreds of years , which is the reason why no or only little toxic effects in humans can be expected. Especially in Africa and Central and South America, traditional medicine is advised by shamans, curanderos, or herbalists who often keep the use of the healing plants as a secret . Although these plants are used since ages, little is known about the “pinciples of activity” and/or the targeted cellular mechanisms, and hence, these remedies have a great potential for drug development. We aimed for the separation and isolation of distinct properties of the Maya healing plant Pluchea odorata which are relevant for anticancer treatment. P. odorata grows in the USA, Mexico, Belize, Guatemala, Panama, Cayman Islands, Guadeloupe, Jamaica, Puerto Rico, St. Lucia, Venezuela, and Ecuador (Germplasm Resources Information Network, United States Department of Agriculture, 9 November 2004, http://www.ars-grin.gov/cgi-bin/npgs/html/taxon.pl?104497) and is still used by the Maya to treat common cold, fever, flu, head colds, headache, hypertension, neuralgia, ophthalmia, palsy, pneumonia, snake bite, swellings, inflammation, and bruises of the skin . The medical solution is prepared by boiling two handfuls of leaves in one gallon of water, and then it is frequently applied on the affected area until the inflammation subsides . Further the plant is described as being antidote, astringent, diaphoretic, and haemostatic , as well as traditionally used by mothers after giving birth to decrease the risk for infections and conveyance of tissue recovery . Gridling et al.  and Bauer et al.  describe a strong anti-neoplastic effect of the dichloromethane extract in HL60 and MCF-7 cells and an anti-inflammatory response in HUVECs (human umbilical vein endothelial cells).
Pharmaceutical drugs are prepared under standardised conditions and usually contain just one active principle. In contrast, ethnopharmacologic remedies are mixtures of a vast number of compounds, which are in many cases unknown, and vary in their composition and activity depending on the growth area and the time of collection. This makes them difficult for application and trading. Moreover, plant extracts can also contain compounds that are systemically toxic or counteract the desired effect of the active principle(s). On the other hand, some of the different compounds in a plant extract can synergise. The present work will give examples of this phenomenon. A common reason to terminate a priori successful therapies of all kinds of cancer and other diseases is the acquisition of drug resistance. However, it has not been reported so far that complex plant mixtures induce treatment resistances in patients, most likely because several distinct active principles target various intra- and intercellular signalling pathways simultaneously thereby preventing that the organism develops an “escape mechanism.” Thus, the development of complex extracts should be considered as a strategy to treat cancer. Standardisation procedures for such mixtures must be individually developed to provide therapeutics which are effective and safe and do not exhibit batch to batch variations. The fractionation and accompanying testing in bioassays and by appropriate analyses are a feasible concept for standardisation and remedies emerging along such procedures can be approved by national agencies (i.e., Avemar, WO 2004014406 (A1): “Use of a fermented wheat germ extract as anti-inflammatory agent” by Hidvegi and Resetar).
Here we describe a fractionation approach of the dichloromethane extract of P. odorata, which was constantly controlled regarding its activity by bio-assays and analyses that can be standardised. This resulted in fractions causing distinct cellular responses indicative for wound healing or anti-neoplastic properties.
2. Material and Methods
2.1. Plant Material
The aerial parts (leaves, caulis, florescence) of Pluchea odorata (L.) Cass. were collected in Guatemala, Departamento Petén, near the north-western shore of Lago Petén Itzá, San José, within an area of four-year-old secondary vegetation ~1 km north of the road from San José to La Nueva San José (16° N, 89° W). Voucher specimens (leg. G. Krupitza & R. O. Frisch, Nr. 1-2009, 08. 04. 2009, Herbarium W) were archived at the Museum of Natural History, Vienna, Austria. 6 kg of air-dried plant material has been extracted with dichloromethane by Björn Feistel (Finzelberg GmbH & Co. KG, Andernach, Germany), and the extract stored in an exsiccator in the dark at 4°C until use.
2.2. Plant Extraction and Fractionation
Plant extraction with dichloromethane was essentially as described earlier [6, 7]. 6000 g dried plant material was extracted with dichloromethane resulting in 220 g dry extract (extraction was performed by Finzelberg GmbH & Co. KG, Andernach, Germany).
Vacuum Liquid Chromatography (VLC) was used for the separation of large amounts of extract. 36 g dichloromethane extract was redissolved in dichloromethane, mixed with 70 g silica gel and evaporated to dryness, and ground in a mortar to obtain a homogenous powder. A 12 × 40 cm column was packed with 900 g silica gel, on top the silica gel-containing extract, and covered with sea sand to ballast the sample. The mobile phase was passed through by application of reduced pressure. After checking the collected fractions by TLC, those with similar bands were recombined, and this resulted in three combined fractions (F1.1–F1.3; Table 1).
VLC Fractionation of F1.1. 10 g of F1.1, which was derived from the crude extract, was dissolved in dichloromethane, mixed with 20 g silica gel, evaporated to dryness, refined in a mortar, and applied on top of a 5 × 60 cm silica gel column. Compounds were eluted with the mobile phases shown in Table 2 by applying reduced pressure. Collected fractions were checked by TLC, and similar fractions were recombined yielding nine combined fractions (F2.1–F2.9).
Column Chromatography (CC) Fractionation of F2.6 (Less Than 2 g of Residue was fractionated by CC). 1.6 g F2.6, which was gained by fractionation of F1.1 was dissolved in dichloromethane, mixed with 3 g silica gel, evaporated to dryness, placed on top of a 5 × 50 cm silicia gel column and eluted with mobile phases shown in Table 3. The collected fractions were checked by TLC and those with similar band patterns were recombined to yield ten combined fractions (F3.1–F3.10).
CC Fractionation of F3.3. 1.08 g of F3.3, which was derived from F2.6, was dissolved in dichloromethane and placed on top of a 2 × 30 cm silica gel column. Mobile phases were used as illustrated in Table 4. Fractions were checked by TLC, and those with similar band patterns were recombined yielding twelve combined fractions (F4.3.1–F4.3.12).
CC Fractionation of F4.3.7. 146 mg F4.3.7 was dissolved dichloromethane and applied on a 80 × 1.5 cm silica gel column and fractionated with one litre solvent (chloroform: methanol: water, 95 : 1.5 : 0.1). Fractions were collected in tubes, ten drops per minute, and every 30 minutes the tubes were changed. Afterwards the column was washed with 300 mL methanol. Fractions were checked by TLC, and those with similar band patterns were recombined resulting in twelve fractions (F184.108.40.206–F220.127.116.11; see Figure 3(c)).
CC Fractionation of F3.6. 0.32 g F3.6, which was derived from F2.6, was dissolved in methanol and applied on top of a 3.5 × 40 cm Sephadex column (2.5 × 40 cm for 3.6). Methanol was used as mobile phase, and fractions were collected and checked by TLC, and those with similar band patterns were recombined to yield four combined fractions: F4.6.1 (9 mg), F4.6.2 (5 mg), F4.6.3 (207 mg), F4.6.4 (55 mg).
CC Fractionation of F4.6.3. 20 mg F4.6.3 (very oily), which was derived from F3.6, was dissolved in dichloromethane, mixed with silica gel, and applied on top a 2.5 × 15 cm dichloromethane conditioned silica gel column. Successful elution was achieved with dichloromethane : ethylacetate (50 : 50). Fractions were checked by TLC and those with similar band patterns were recombined yielding six combined fractions (F18.104.22.168–F22.214.171.124; see Figure 4(b)).
2.3. Thin Layer Chromatography (TLC)
TLC was used for control of fractionation. Stationary phase and mobile phases are described in Table 5. The mobile phase varied between five solvent systems. Plates were detected under UV254, UV366, and visible light, before and after spraying with anisaldehyde sulphuric acid reagent (ASR). ASR consisted of 0.5 mL anisaldehyde, 10 mL glacial acetic acid, 85 mL methanol and 5 mL H2SO4 (sulfuric acid). The sprayed plate was heated at 100°C for five minutes, and then compounds were detected under UV254,365 and visible light. Unless otherwise stated 8 μL extract or fraction solution was applied to the plate.
2.4. Cell Culture
HL-60 (human promyelocytic leukaemia cell) cells were purchased from American Type Culture Collection (ATCC). The cells were grown in RPMI 1640 medium which was supplemented with 10% heat-inactivated fetal calf serum (FCS), 1% Glutamax, and 1% Penicillin-Streptomycin. Both medium and supplements were obtained from Life Technologies (Carlsbad, CA, USA). The cells were kept in humidified atmosphere at 37°C containing 5% CO2.
2.5. Proliferation Assay
Proliferation assays [8, 9] were performed to analyse the inhibition of proliferation of HL-60 cells treated with extract or fractions of P. odorata. Extract and fractions were dissolved in ethanol (final concentration was 0.2%). HL-60 cells were seeded in 24-well plates at a concentration of 1 × 105 cells per mL RPMI medium allowing logarithmic growth within the time of treatment with plant extract or fractions. The control was treated with solvent. After 24 and 48 hours, the number of cells was determined using the Sysmex Cell Counter (Sysmex Corp., Kobe, Japan). Experiments were done in triplicate. Percentage of cell division progression compared to the untreated control was calculated by applying the following formula:
2.6. Apoptosis Assay
Determination of cell death by Hoechst 33258 (HO) and propidium iodide (PI) double staining (both Sigma, St. Louis, MO, USA) allows identifying the amount and the type of cell death (early or late apoptosis or necrosis) [10–12]. Therefore, HL-60 cells were seeded in a 24-well plate at a concentration of 1 × 105 cells per mL RPMI medium. Cells were treated with fractions or extract of P. odorata. The cells were incubated for 8, 24, 48, and/or 72 hours, depending on the experiment. At each time point, 100 μL cell suspension of each well was transferred into separate wells of a 96-well plate, and Hoechst 33285 and propidium iodide were added at final concentrations of 5 μg/mL and 2 μg/mL, respectively. After one hour of incubation at 37°C, stained cells were examined and photographed with an Axiovert fluorescence microscope (Zeiss, Jena, Germany) equipped with a DAPI filter. Type and number of cell deaths were evaluated by visual examination of the photographs according to the morphological characteristics revealed by HOPI staining. Experiments were done in triplicate.
2.7. Western Blotting
Preparation of lysates. HL60 cells were seeded in a tissue culture flask at a concentration of 1 × 106 cells per mL RPMI medium. P. odorata fractions F1, F4.6.3, and F4.3.7 were analysed by western blots. HL60 cells were either incubated with 40 μg/mL F1 or with 10 μg/mL of one of the other two P. odorata fractions for the indicated times. At each time point, 4 × 106 cells were harvested, placed on ice, and centrifuged (1000 rpm, 4°C, 4 min). Then, the supernatant (medium) was discarded, and the pellet was washed twice with cold phosphate buffered saline (PBS, pH 7.2) and centrifuged (1000 rpm, 4°C, 4 min). The cell pellet was lysed in a buffer containing 150 mM NaCl, 50 mM Tris (pH 8.0), 1% Triton-X-100, 1 mM phenylmethylsulfonyl fluoride (PMSF), and 1 mM protease inhibitor cocktail (PIC) (Sigma, Schnelldorf, Germany). Afterwards the lysate was centrifuged at 12000 rpm for 20 min at 4°C. Supernatant was transferred into a 1.5 mL tube and stored at −20°C for further analyses.
Gel electrophoresis (SDS-PAGE) and blotting. Equal amounts of protein samples (lysate) were mixed with sodium dodecyl sulfate (SDS) sample buffer (1 : 1) and loaded onto a 10% polyacrylamide gel. Proteins were separated by polyacrylamide gel electrophoresis (PAGE) at 120 Volt for approximately one hour. To make proteins accessible to antibody detection, they were electrotransferred from the gel onto a polyvinylidene difluoride (PVDF) Hybond membrane (Amersham, Buckinghamshire, UK) at 95 Volt for 80 minutes. Membranes were allowed to dry for 30 minutes to provide fixing of the proteins on the membrane. Methanol was used to moist the membranes. Equal sample loading was checked by staining the membrane with Ponceau S (Sigma, Schnelldorf, Germany).
Protein detection. After washing with PBS or TBS (Tris buffered saline, pH 7.6), membranes were blocked in PBS- or TBS-milk (5% nonfat dry milk in PBS containing 0.5% Tween 20 or TBS containing 0.1% Tween 20) for one hour at room temperature. Then membranes were washed with PBS/T (PBS containing 0.5% Tween 20) or TBS/T (TBS containing 0.1% Tween 20), changing the washing solution four to five times every five minutes. Then every membrane was incubated with a primary antibody (1 : 500) in blocking solution (according to the data sheet TBS-, PBS-milk or TBS-, PBS-BSA), at 4°C over night gently shaking. Subsequently the membrane was again washed with PBS/T or TBS/T and incubated with the second antibody (peroxidase-conjugated goat anti-rabbit IgG or anti-mouse IgG) diluted 1 : 2000 for one hour at room temperature. After washing the membranes, chemiluminescence was developed with enhanced chemiluminescence (ECL) plus detection kit (Amersham, UK) (two seconds to ten minutes), and membranes were exposed to the Lumi-Imager F1 (Roche) for increasing times.
Monoclonal mouse ascites fluid anti-acetylated α-tubulin (6-11B-1) and β actin (AC-15) antibodies were from Sigma (St. Louis, MO, USA). Monoclonal mouse α-tubulin (DM1A), β-tubulin (H-235), Cdc25A (F-6), and polyclonal rabbit paxillin (H-114), ROCK-1 (C8F7), c-Jun (H-79), Jun b (210) were from Santa Cruz Biotechnology, Inc. (Santa Cruz, CA, USA). Monoclonal rabbit cleaved caspase 8 (Asp391) (18C8) and phospho-Stat3 (Tyr705)(D3A7) antibodies and polyclonal rabbit cleaved caspase 3 (Asp175), human-specific cleaved caspase 9 (Asp330), phospho-Chk2 (Thr68), Chk2, phospho-myosin light chain 2 (MLC2-Ser19), myosin light chain 2, Stat3, and MYPT1 were from Cell Signaling (Danvers, MA, USA). Polyclonal rabbit phospho-Cdc25A (Ser177) antibody was from Abgent (San Diego, CA, USA), polyclonal rabbit phospho-MYPT1 (Thr696) from Upstate (NY, USA), mouse monoclonal γH2AX (pSer139) (DR 1017) from Calbiochem (San Diego, CA, USA), and mouse monoclonal c-Myc Ab-2 (9E10.3) from Thermo Fisher Scientific, Inc. (Fremont, CA, USA). The secondary antibodies peroxidase-conjugated anti-rabbit IgG and anti-mouse IgG were purchased from Dako (Glostrup, Denmark).
2.9. Statistical Analysis
For statistical analyses, Excel 2003 software and Prism 5 software package (GraphPad, San Diego, CA, USA) were used. The values were expressed as mean ± standard deviation, and Student’s -test was applied to compare differences between control samples and treatment groups. Statistical significance level was set to .
3. Results and Discussion
The dichloromethane extract of P. odorata exhibits strong anti-neoplastic activity (Figure 1(a)). Therefore, we fractionated this extract and constantly monitored the activities by bio-assays measuring apoptosis and/or proliferation rates to get closer to the active principles. In the first round the crude extract was split in three distinct fractions of which fraction F1.1 exhibited the strongest anti-proliferative and proapoptotic activity (Figures 1(b) and 1(c)). 40 μg F1.1/mL induced caspase 3 and decreased β-actin and α-tubulin levels, and therefore also reduced acetylation levels of α-tubulin were detected within 4 h of treatment (Figure 1(d)). This suggested that the overall protein decrease was due to the early activation of caspase 3 and subsequent cell death.
F1.1 was further processed yielding fractions F2.1–F2.9. F2.6 was nearly as active F2.7 (Figure 2(a)) but contained ~10 times more fraction material (1.9 g versus 0.2 g, resp.). Therefore, F2.6 was further processed yielding fractions F3.1–F3.10 (Figures 2(b) and 2(c)).
10 μg/mL of F3.4–F3.6 exhibited potent anti-proliferative properties in HL60 cells suppressing cell growth by 100%. The TLC analysis showed that both, F3.3 and F3.6, contained a distinct main compound, and therefore F3.3 and F3.6 were further fractionated. Also F3.2 was processed, however, this yielded only several low-activity fractions (data not shown). (i)The subfractionation of F3.3 on a silica gel column yielded the potent antiproliferative and proapoptotic fraction F4.3.7 (Figures 3(a) and 3(b)). Further fractionation of F4.3.7 caused the decomposition of the strong cytotoxic activity into many low active fractions (F126.96.36.199–F188.8.131.52; Figure 3(c)), which in sum approximated the activity of the precursor. (ii)The subprocessing of F3.6 yielded fractions F4.6.1–F4.6.4. F4.6.3, which was very oily, was the most pro-apoptotic one (Figure 4(a)). Upon further fractionation, the activity of F4.6.3 also decomposed into several low-activity fractions (F184.108.40.206–F220.127.116.11; Figure 4(b)).
Therefore, we went back to F4.3.7 and F4.6.3 and continued analyses with these two distinct high-activity fractions. The TLC patterns of F4.3.7 and F4.6.3 were clearly different from each other evidencing that they contain different compounds (Figure 5(a)). To characterise the two distinct fraction types, posttranslational modifications and expression levels of proteins, which are relevant for apoptosis and cell cycle arrest, were investigated. F4.3.7 slightly induced Chk2 phosphorylation and hence its activation, whereas F4.6.3 did not (Figure 5(b)). Chk2 was shown to phosphorylate Cdc25A at Ser177 and tags it for proteasomal degradation [13, 14]. However, treatment of HL60 cells with F4.3.7 caused the dephosphorylation of Ser177 and protein stabilisation. Also F4.6.3 stabilised Cdc25A despite Ser177 phosphorylation. This implicated that Cdc25A was not regulated by Chk2 activity in this scenario. Moreover Cdc25A stabilisation suggested an increase in cell cycle activity . Nevertheless, cell proliferation was inhibited.
In search of molecular causes for reduced proliferation, we found that the fractionation steps enriched a spindle toxin or an indirect microfilament-targeting activity. This was reflected by induced α-tubulin acetylation, which is an indicator of the polymerisation status of tubulin microfilaments [16, 17], within 2 h of treatment with F4.3.7 and F4.6.3 (Figure 5(c)). Thereafter, caspase 3 became activated. Also the phosphorylation of H2AX occurred after treatment with both fractions indicating DNA damage presumably due to caspase-3-induced DNase activity of DNA fragmentation factor (DFF; ), because caspase 3 activation and H2AX phosphorylation appeared simultaneously . Evidently, the molecular onset of apoptosis occurred faster than the orchestrated expression of the investigated cell cycle regulators. Interestingly, the activation of caspase 3 concurred with the activation of caspase 8, but not with activation of caspase 9, indicating that the extrinsic apoptosis pathway became activated and not the intrinsic one. The signature-type processing of caspase 3 into the active fragment was more prominent by F1.1 than by F4.3.7 and F4.6.3. This was most likely due to the four times higher F1.1 concentration used (40 μg/mL), which caused also the degradation of α-tubulin and β-actin as consequence of swift onset of cell death.
The low or absent activation of Chk2 (resp.) suggested that a genotoxic activity, which was formerly present in the crude extract  and in other subfractions , was eliminated throughout the described fractionations. Avoiding genotoxicity can be beneficial, because it reduces DNA damage and subsequent mutations that may cause secondary malignancies. Cdc25A, a classified oncogene [20, 21] was upregulated by both fraction types and therefore we investigated also the expression of other oncogenes, which are related to tumour growth and progression. F4.6.3 had a substantial effect on the repression of c-Myc and only a minor effect on c-Jun. Even more effective F4.3.7 suppressed also the phosphorylation of Tyr705 of Stat3 and thus inhibited its function, which is known to play a role in tumour progression . This fraction further repressed JunB, c-Jun, and c-Myc more effectively than F4.6.3.
Since P. odorata is used also as a wound healing remedy, this property also involves tissue regeneration and the regulation of a process called “epithelial to mesenchymal transition” (EMT) [23, 24]. The most prominent feature of EMT is the acquisition of a mobile phenotype [25, 26]. If transient and tightly regulated, EMT is beneficial for the organism, because it contributes to acute inflammation and tissue repair [27–29]. In contrast, the chronic status occurrence of EMT causes pathologies such as progression of cancer . The mobility of cancer cells is a prerequisite for the intra- and extravasation of the vasculature, tissue invasion, and metastatic spread [23, 31], and it is mediated by proteins that allow cell plasticity and movement. Therefore, the alteration of motility-related gene products in cancerous cells, such as paxillin [32, 33], ROCK1 , MLC2 for the formation of stress fibres  and MYPT , are indicators for increased mobility and hence cancer progression. Also leukaemia cells such as differentiated HL60 attach to the ECM and vascular cells and transmigrate through vessel walls, invade tissues [37–39], and add to the progression of the disease. Hence, HL60 cells possess a repertoire of proteins facilitating cell movement although they normally grow in suspension. Treatment with F4.3.7 caused ROCK1 repression below constitutive and detectable levels, which was not the case with F4.6.3 (Figure 5(d)). Also MYPT expression decreased upon treatment with F4.3.7. Paxillin became upregulated by F4.6.3 treatment and marginally by F4.3.7, and this was also the case for the phosphorylation of MLC2. Since P. odorata is successfully used for tissue recovery and healing of skin bruises, the increased mobility of cells (fibroblasts, epithelial cells, macrophages, etc.) is required to close the tissue disruption. This very property, however, is detrimental throughout cancer treatment, and elimination of this activity might be beneficial for this purpose. Therefore, future research has to address the question whether F4.3.7 is advantageous for cancer cell treatment, whereas F4.6.3 exhibits advanced wound healing properties.
A spindle-damaging activity became enriched by fractionations, which was reflected by increased α-tubulin acetylation followed by the activation of caspases 8 and 3 and the typical nuclear morphology of apoptosis. The impact on apoptosis and the orchestration of apoptosis regulator activation were similar for both fractions. In comparison to earlier work, genotoxic components activating Chk2 were eliminated.
Importantly, F4.6.3 induced mobility markers, whereas F4.3.7 inhibited the expression of mobility markers or did not interfere with their constitutive expression. This property implicates an inhibitory effect of F4.3.7 on tumour progression which was also reflected by the downregulation of the Jun family of oncogenes and the suppression of Stat3 activity.
These findings can provide a basis for the development of remedies (1) supporting wound healing in case of F4.6.3 or (2) interfering with tumour progression in case of F4.3.7.
The authors wish to thank Toni Jäger for preparing the figures. This work was supported by the Funds for Innovative and Interdisciplinary Cancer Research to G. Krupitza.
- D. S. Fabricant and N. R. Farnsworth, “The value of plants used in traditional medicine for drug discovery,” Environmental Health Perspectives, vol. 109, no. 1, pp. 69–75, 2001.
- R. P. Rastogi and B. N. Dhawan, “Research on medicinal plants at the Central Drug Research Institute, Lucknow (India),” Indian Journal of Medical Research, vol. 76, pp. 27–45, 1982.
- R. Arvigo and M. Balick, “One hundred healing herbs of Belize,” in Rainforest Remedies, pp. 72–73, Lotus, Twin Lakes, Wis, USA, 2nd edition, 1998.
- M. Balick and R. Lee, “Inflammation and ethnomedicine: looking to our past,” Explore, vol. 1, no. 5, pp. 389–392, 2005.
- T. Johnson, CRC Ethnobotany Desk Reference, CRC Press, Boca Raton, Fla, USA, 1999.
- M. Gridling, N. Stark, S. Madlener et al., “In vitro anti-cancer activity of two ethno-pharmacological healing plants from Guatemala Pluchea odorata and Phlebodium decumanum,” International Journal of Oncology, vol. 34, no. 4, pp. 1117–1128, 2009.
- S. Bauer, J. Singhuber, M. Seelinger et al., “Separation of anti-neoplastic activities by fractionation of a Pluchea odorata extract,” Frontiers in Bioscience, vol. 3, pp. 1326–1336, 2011.
- S. Strasser, S. Maier, C. Leisser et al., “5-FdUrd-araC heterodinucleoside re-establishes sensitivity in 5-FdUrd- and AraC-resistant MCF-7 breast cancer cells overexpressing ErbB2,” Differentiation, vol. 74, no. 9-10, pp. 488–498, 2006.
- Y. Bader, S. Madlener, S. Strasser et al., “Stillbene analogues affect cell cycle progression and apoptosis independently of each other in an MCF-7 array of clones with distinct genetic and chemoresistant backgrounds,” Oncology Reports, vol. 19, no. 3, pp. 801–810, 2008.
- A. Ozmen, S. Madlener, S. Bauer et al., “In vitro anti-leukemic activity of the ethno-pharmacological plant Scutellaria orientalis ssp. carica endemic to western Turkey,” Phytomedicine, vol. 17, no. 1, pp. 55–62, 2010.
- S. Maier, S. Strasser, P. Saiko et al., “Analysis of mechanisms contributing to AraC-mediated chemoresistance and re-establishment of drug sensitivity by the novel heterodinucleoside phosphate 5-FdUrd-araC,” Apoptosis, vol. 11, no. 3, pp. 427–440, 2006.
- G. Rosenberger, G. Fuhrmann, M. Grusch et al., “The ribonucleotide reductase inhibitor trimidox induces c-myc and apoptosis of human ovarian carcinoma cells,” Life Sciences, vol. 67, no. 26, pp. 3131–3142, 2000.
- S. Madlener, M. Rosner, S. Krieger et al., “Short 42°C heat shock induces phosphorylation and degradation of Cdc25A which depends on p38MAPK, Chk2 and 14.3.3,” Human Molecular Genetics, vol. 18, no. 11, pp. 1990–2000, 2009.
- C. Karlsson-Rosenthal and J. B. A. Millar, “Cdc25: mechanisms of checkpoint inhibition and recovery,” Trends in Cell Biology, vol. 16, no. 6, pp. 285–292, 2006.
- I. Blomberg and I. Hoffmann, “Ectopic expression of Cdc25A accelerates the G1/S transition and leads to premature activation of cyclin E- and cyclin A-dependent kinases,” Molecular and Cellular Biology, vol. 19, no. 9, pp. 6183–6194, 1999.
- G. Piperno, M. LeDizet, and X. J. Chang, “Microtubules containing acetylated alpha-tubulin in mammalian cells in culture,” The Journal of Cell Biology, vol. 104, no. 2, pp. 289–302, 1987.
- C. Hubbert, A. Guardiola, R. Shao et al., “HDAC6 is a microtubule-associated deacetylase,” Nature, vol. 417, no. 6887, pp. 455–458, 2002.
- X. Liu, H. Zou, C. Slaughter, and X. Wang, “DFF, a heterodimeric protein that functions downstream of caspase-3 to trigger DNA fragmentation during apoptosis,” Cell, vol. 89, no. 2, pp. 175–184, 1997.
- T. T. Paull, E. P. Rogakou, V. Yamazaki, C. U. Kirchgessner, M. Gellert, and W. M. Bonner, “A critical role for histone H2AX in recruitment of repair factors to nuclear foci after DNA damage,” Current Biology, vol. 10, no. 15, pp. 886–895, 2000.
- H. Kiyokawa and D. Ray, “In vivo roles of CDC25 phosphatases: biological insight into the anti-cancer therapeutic targets,” Anti-Cancer Agents in Medicinal Chemistry, vol. 8, no. 8, pp. 832–836, 2008.
- D. Ray and H. Kiyokawa, “CDC25A phosphatase: a rate-limiting oncogene that determines genomic stability,” Cancer Research, vol. 68, no. 5, pp. 1251–1253, 2008.
- E. Devarajan and S. Huang, “STAT3 as a central regulator of tumor metastases,” Current Molecular Medicine, vol. 9, no. 5, pp. 626–633, 2009.
- F. van Zijl, G. Krupitza, and W. Mikulits, “Initial steps of metastasis: cell invasion and endothelial transmigration,” Mutation Research, vol. 728, no. 1-2, pp. 23–34, 2011.
- J. P. Thiery, H. Acloque, R. Y. J. Huang, and M. A. Nieto, “Epithelial-mesenchymal transitions in development and disease,” Cell, vol. 139, no. 5, pp. 871–890, 2009.
- R. Kalluri and R. A. Weinberg, “The basics of epithelial-mesenchymal transition,” The Journal of Clinical Investigation, vol. 119, no. 6, pp. 1420–1428, 2009.
- C. Vonach, K. Viola, B. Giessrigl et al., “NF-κB mediates the 12(S)-HETE-induced endothelial to mesenchymal transition of lymphendothelial cells during the intravasation of breast carcinoma cells,” British Journal of Cancer, vol. 105, no. 2, pp. 263–271, 2011.
- H. Lu, W. Ouyang, and C. Huang, “Inflammation, a key event in cancer development,” Molecular Cancer Research, vol. 4, no. 4, pp. 221–233, 2006.
- S. I. Grivennikov, F. R. Greten, and M. Karin, “Immunity, inflammation, and cancer,” Cell, vol. 140, no. 6, pp. 883–899, 2010.
- J. M. López-Nouoa and M. A. Nieto, “Inflammation and EMT: an alliance towards organ fibrosis and cancer progression,” EMBO Molecular Medicine, vol. 1, no. 6-7, pp. 303–314, 2009.
- Y. Wu and B. P. Zhou, “Inflammation: a driving force speeds cancer metastasis,” Cell Cycle, vol. 8, no. 20, pp. 3267–3273, 2009.
- G. Krupitza, S. Grill, H. Harant et al., “Genes related to growth and invasiveness are repressed by sodium butyrate in ovarian carcinoma cells,” British Journal of Cancer, vol. 73, no. 4, pp. 433–438, 1996.
- M. D. Schaller, “Paxillin: a focal adhesion-associated adaptor protein,” Oncogene, vol. 20, no. 44, pp. 6459–6472, 2001.
- N. O. Deakin and C. E. Turner, “Paxillin comes of age,” Journal of Cell Science, vol. 121, part 15, pp. 2435–2444, 2008.
- E. Sahai and C. J. Marshall, “Differing modes for tumour cell invasion have distinct requirements for Rho/ROCK signalling and extracellular proteolysis,” Nature Cell Biology, vol. 5, no. 8, pp. 711–719, 2003.
- G. Totsukawa, Y. Yamakita, S. Yamashiro, D. J. Hartshorne, Y. Sasaki, and F. Matsumura, “Distinct roles of ROCK (Rho-kinase) and MLCK in spatial regulation of MLC phosphorylation for assembly of stress fibers and focal adhesions in 3T3 fibroblasts,” The Journal of Cell Biology, vol. 150, no. 4, pp. 797–806, 2000.
- S. Vetterkind, E. Lee, E. Sundberg et al., “Par-4: a new activator of myosin phosphatase,” Molecular Biology of the Cell, vol. 21, no. 7, pp. 1214–1224, 2010.
- P. Liu, J. Li, H. Lu, and B. Xu, “Thalidomide inhibits leukemia cell invasion and migration by upregulation of early growth response gene 1,” Leukemia and Lymphoma, vol. 50, no. 1, pp. 109–113, 2009.
- L. Wang, J. Learoyd, Y. Duan, A. R. Leff, and X. Zhu, “Hematopoietic Pyk2 regulates migration of differentiated HL-60 cells,” Journal of Inflammation, vol. 7, article 26, 2010.
- D. Raman, J. Sai, N. F. Neel, C. S. Chew, and A. Richmond, “LIM and SH3 protein -1 modulates CXCR2-mediated cell migration,” PLoS One, vol. 5, no. 4, Article ID e10050, 2010.