Baixe o app para aproveitar ainda mais
Prévia do material em texto
The bioenergetics of cancer: Is glycolysis the main ATP supplier in all tumor cells? Rafael Moreno-Sánchez,* Sara Rodrı́guez-Enrı́quez, Emma Saavedra, Alvaro Marı́n-Hernández, Juan Carlos Gallardo-Pérez Instituto Nacional de Cardiologı́a, Departamento de Bioquı́mica, Juan Badiano 1, Tlalpan, México DF, Mexico Abstract. The molecular mechanisms by which tumor cells achieve an enhanced glycolytic flux and, presumably, a decreased oxidative phosphorylation are analyzed. As the O2 concentration in hypoxic regions of tumors seems not limiting for oxidative phosphorylation, the role of this mitochondrial pathway in the ATP supply is re-evaluated. Drugs that inhibit glycoysis and oxidative phosphorylation are analyzed for their specificity toward tumor cells and effect on proliferation. The energy metabolism mechanisms involved in the use of positron emission tomography are revised and updated. It is proposed that energy metabolism may be an alternative therapeutic target for both hypoxic (glycolytic) and oxidative tumors. VC 2009 International Union of Biochemistry and Molecular Biology, Inc. Volume 35, Number 2, March/April 2009, Pages 209–225 � E-mail: rafael.moreno@cardiologia.org.mx or morenosanchez@hotmail.com Keywords: glycolysis, oxidative phosphorylation, mitochondrial function, PET, metabolic control analysis 1. Introduction All tumor cell types show an altered energy metabolism in comparison to their tissue of origin (Figs. 1 and 2). The best characterized energy metabolism modification in tumor cells is an increased glycolytic capacity even in the presence of a high O2 concentration ([1], reviewed in ref. 2). Several mech- anisms for the enhanced glycolysis in tumor cells have been proposed (Table 1). However, each particular tumor cell line has its own combination of mechanisms to increase glycoly- sis and, therefore, generalizations should be avoided. 2. Genetic regulation of glycolysis In tumor cells, there is an enhanced transcription of genes of several or all glycolytic pathway enzymes and transport- ers that is accompanied by an enhanced protein synthesis [2]. It is usually assumed that these transcriptional changes lead to increased activity and pathway flux. Unfortunately, the required biochemical (metabolic, kinetic) experimenta- tion is considered ‘‘old-fashioned’’ and, only in few of the molecular biology studies, transporter and enzyme activities and flux rate have been determined. In comparison with normal rat hepatocytes, the activity of all glycolytic enzymes are overexpressed in rat AS-30D hepatoma by 2–4 times (HPI, ALD, TPI, GAPDH, PGK, PGAM, ENO, and LDH), 8- to 10-fold for PYK, and 17–300 times for PFK-1 and HK (Fig. 1) [10]. For human cervix HeLa cells, all enzymes including HK and PFK-1 are overexpressed by 2–7 times, with the exception of PGAM and LDH which are 2–7 times lower than in rat hepatocytes [10]. However, for this last case a more rigorous comparison should be made with normal uterine cervix epithelial cells, the original source, when data become available. In rat Morris hepatomas, the activities of HK, PFK and PYK are 5- to 500-fold higher than in liver [26], whereas in human breast cancer, the activities of HK, ALD, PYK, and LDH are 3.7–7 times higher than in normal tissue [27]. In several human carcinomas, overexpres- sion (Table 1) of GLUT [3], GAPDH, ENO-1, PYK, and LDH [28,29], correlates with a high glycolysis rate. In contrast, in human cartilage and bone marrow cancer, glycolysis is high but only sporadic expression of GAPDH, ENO-1, and PYK is observed [29]. Unfortunately, the expression pattern of the whole set of glycolytic enzymes is not always analyzed, which frequently leads to extend these observations to all types of cancer. In cancer cells, the hypoxia inducible factor 1a (HIF-1a) is a transcriptional factor that upregulates the expression of specific isoforms of GLUT, HK, PFK-1, PFK-2, ALD, GAPDH, Abbreviations: ALD, aldolase; AcCoA, acetyl CoA; Cit, citrate; DHAP, dihydroxyacetone phosphate; ENO, enolase; F6P, fructose-6-phosphate; F1,6BP, fructose-1, 6- bisphosphate; F2,6BP, fructose-2, 6-bisphosphate; Fum, fumarate; GAPDH, glyceraldehyde-3-phosphate dehydrogenase; aGPDH, a-glycerophosphate dehydrogenase; GLUT, glucose transporter; G6P, glucose-6-phosphate; Gln, glutamine; Glut, glutamate; HK, hexokinase; HPI, hexose-6-phosphate isomerase; LDH, lactate dehydrogenase; OxPhos, oxidative phosphorylation; 2-Oxo, 2-oxoglutarate; PDH, pyruvate dehydrogenase complex; PET, positron energy transfer; PFK-1, phosphofructokinase type 1; PGK, phosphoglycerate kinase; PGAM, phosphoglycerate mutase; PYK, pyruvate kinase; PEP, phosphoenolpyruvate; 1,3 BPG, 1,3- bisphosphoglycerate; 2PG, 2-phosphoglycerate; 3PG, 3 phosphoglycerate; Pyr, pyruvate;TPI, triosephosphate isomerase. *Address for correspondence: Rafael Moreno-Sánchez, Ph.D., Instituto Nacional de Cardiologı́a, Departamento de Bioquı́mica, Juan Badiano No. 1, Col. Seccion XVI, Tlalpan, México DF 14080, Mexico. Tel: þ5255 5573 2911 (ext. 1422, 1298); E-mail: rafael.moreno@cardiologia.org.mx or morenosanchez@hotmail.com. Received 3 December 2008; accepted 18 January 2009 DOI: 10.1002/biof.31 Published online 11 March 2009 in Wiley InterScience (www.interscience.wiley.com) 209 https://www.researchgate.net/publication/6502225_Energy_metabolism_in_tumor_cells_FEBS_J?el=1_x_8&enrichId=rgreq-e4392ea4-f659-4597-9cdf-54af3672b40b&enrichSource=Y292ZXJQYWdlOzI0NDM0MzA4O0FTOjEwNDEzMDM2NjQxMDc2NEAxNDAxODM4MDI1NTA2 https://www.researchgate.net/publication/7139756_Determining_and_understanding_the_control_of_glycolysis_in_fast-growth_tumor_cells_Flux_control_by_an_over-expressed_but_strongly_product-inhibited_hexokinase_FEBS_J?el=1_x_8&enrichId=rgreq-e4392ea4-f659-4597-9cdf-54af3672b40b&enrichSource=Y292ZXJQYWdlOzI0NDM0MzA4O0FTOjEwNDEzMDM2NjQxMDc2NEAxNDAxODM4MDI1NTA2 https://www.researchgate.net/publication/7139756_Determining_and_understanding_the_control_of_glycolysis_in_fast-growth_tumor_cells_Flux_control_by_an_over-expressed_but_strongly_product-inhibited_hexokinase_FEBS_J?el=1_x_8&enrichId=rgreq-e4392ea4-f659-4597-9cdf-54af3672b40b&enrichSource=Y292ZXJQYWdlOzI0NDM0MzA4O0FTOjEwNDEzMDM2NjQxMDc2NEAxNDAxODM4MDI1NTA2 https://www.researchgate.net/publication/16614624_Enzyme_activities_in_normal_dysplastic_and_cancerous_breast_tissues?el=1_x_8&enrichId=rgreq-e4392ea4-f659-4597-9cdf-54af3672b40b&enrichSource=Y292ZXJQYWdlOzI0NDM0MzA4O0FTOjEwNDEzMDM2NjQxMDc2NEAxNDAxODM4MDI1NTA2 https://www.researchgate.net/publication/10925652_Understanding_the_Tumor_Metabolic_Phenotype_in_the_Genomic_Era?el=1_x_8&enrichId=rgreq-e4392ea4-f659-4597-9cdf-54af3672b40b&enrichSource=Y292ZXJQYWdlOzI0NDM0MzA4O0FTOjEwNDEzMDM2NjQxMDc2NEAxNDAxODM4MDI1NTA2 https://www.researchgate.net/publication/10267165_On_the_Origin_of_Cancer_Cell?el=1_x_8&enrichId=rgreq-e4392ea4-f659-4597-9cdf-54af3672b40b&enrichSource=Y292ZXJQYWdlOzI0NDM0MzA4O0FTOjEwNDEzMDM2NjQxMDc2NEAxNDAxODM4MDI1NTA2 PGK, PGAM, ENO, PYK, and LDH (Table 1). In consequence, the glycolytic flux and the levels of intermediaries are increased. Notwithstanding the O2 level, metastatic tumor cell lines show high levels of HIF-1a, overexpression of gly- colytic enzymes, and high glycolysis. Nonmetastatic tumor cells increase HIF-1a, enzyme overexpression and glycolysis only under hypoxia [30], although VHL-deficient tumors [31] and tumors with mutations of succinate dehydrogenase or fumarate hydratase (see later) have constitutive and aerobic HIF-1a stabilization. HIF-1a upregulates PDH kinase 1, which inhibits by phosphorylation the PDH complex. As a consequence, it has been proposed that PDH inactivation ocurrs in cancer cells, which leads to decreased pyruvate oxidation through the Krebs cycle and decreased mitochondrial oxygen consump- tion [32,33]. Indeed, overexpression of PDK1 induces an increase of three times in ATP content during hypoxia in the absence of HIF-1a, and knockdown of PDK1 increases respi- ration by 25% during hypoxia [32,33]. This PDK1-mediatedmechanism would impair the mitochondrial function inducing a shift to a glycolytic metabolism in cancer cells. However, this fashionable proposal [34,35] makes several assumptions which have not been experimentally validated. For instance, full PDH phosphorylation and inactivation are not achieved. Neither significant diminution of the respiratory and ATP syn- thesis rates nor, in contrast, a glycolysis enhancement, has been demonstrated. Furthermore, tumor mitochondria are able to oxidize several other substrates such as glutamine, glutamate, fatty acids, and ketone bodies (reviewed in ref. 2) which do not depend on the PDH complex activity. Building theories on metabolic changes in cancer cells based only on transcriptional/proteomic profiling, without making an actual assessment of the function claimed to be affected, although informative, does not allow for a complete understanding of the actual in vivo energy metabolism of cancer cells. Unfortunately, the field is abundant in this type of generalizations. Combination of newly developed experi- mental strategies with classical biochemical and metabolic Fig. 1. Glycolysis in fast-growing cancer cells. In tumor cells, there is over-expression of GLUT1 and GLUT3, HKII (which may bind to the outer mitochondrial membrane, thus readily accessing to the newly synthesized ATP by OxPhos), PFK1, PFK-2FB3, and LDH-A among others. Tumor HK is strongly inhibited by its product G6P, whereas PFK-1 activation by F2,6BP overcomes the citrate and ATP inhibition. In some tumors, aGPDH is down-regulated. An increased flux towards ribose-5-phosphate (and nucleotides) synthesis is documented for several tumor cells. In addition to be transformed in L-lactate, pyruvate may be oxidized by mitochondria (MIT), generate alanine, and synthesizes malate in a reaction catalyzed by an over-expressed cytosolic malic enzyme. Other relevant branches of the glycolytic pathway are also indicated. Abbreviations: Ala, alanine; ANT, adenine nucleotide translocator; Cys, cysteine; ERI4P, erythrose 4-phosphate; GLU, glucose; Gly, glycine; LAC, lactate; Mal, malate; MCT, monocarboxylate transporter; ME, malic enzyme; Ser, serine; TGs, triglycerides; PM, plasma membrane. [Color figure can be viewed in the online issue, which is available at www.interscience.wiley.com.] 210 BioFactors https://www.researchgate.net/publication/12212933_Krieg_M_Haas_R_Brauch_H_Acker_T_Flamme_I_and_Plate_KH_Up-regulation_of_hypoxia-inducible_factors_HIF-1_and_HIF-2_under_normoxic_conditions_in_renal_carcinoma_cells_by_von_Hippel-Lindau_tumor_suppresso?el=1_x_8&enrichId=rgreq-e4392ea4-f659-4597-9cdf-54af3672b40b&enrichSource=Y292ZXJQYWdlOzI0NDM0MzA4O0FTOjEwNDEzMDM2NjQxMDc2NEAxNDAxODM4MDI1NTA2 https://www.researchgate.net/publication/7261461_Papandreou_I_Cairns_RA_Fontana_L_Lim_AL_Denko_NC_HIF-1_mediates_adaptation_to_hypoxia_by_actively_downregulating_mitochondrial_oxygen_consumption_Cell_Metab_3_187-197?el=1_x_8&enrichId=rgreq-e4392ea4-f659-4597-9cdf-54af3672b40b&enrichSource=Y292ZXJQYWdlOzI0NDM0MzA4O0FTOjEwNDEzMDM2NjQxMDc2NEAxNDAxODM4MDI1NTA2 https://www.researchgate.net/publication/7261461_Papandreou_I_Cairns_RA_Fontana_L_Lim_AL_Denko_NC_HIF-1_mediates_adaptation_to_hypoxia_by_actively_downregulating_mitochondrial_oxygen_consumption_Cell_Metab_3_187-197?el=1_x_8&enrichId=rgreq-e4392ea4-f659-4597-9cdf-54af3672b40b&enrichSource=Y292ZXJQYWdlOzI0NDM0MzA4O0FTOjEwNDEzMDM2NjQxMDc2NEAxNDAxODM4MDI1NTA2 https://www.researchgate.net/publication/5314945_Pyruvate_Dehydrogenase_Complex_Activity_Controls_Metabolic_and_Malignant_Phenotype_in_Cancer_Cells?el=1_x_8&enrichId=rgreq-e4392ea4-f659-4597-9cdf-54af3672b40b&enrichSource=Y292ZXJQYWdlOzI0NDM0MzA4O0FTOjEwNDEzMDM2NjQxMDc2NEAxNDAxODM4MDI1NTA2 https://www.researchgate.net/publication/6579004_A_Mitochondria-K_Channel_Axis_Is_Suppressed_in_Cancer_and_Its_Normalization_Promotes_Apoptosis_and_Inhibits_Cancer_Growth?el=1_x_8&enrichId=rgreq-e4392ea4-f659-4597-9cdf-54af3672b40b&enrichSource=Y292ZXJQYWdlOzI0NDM0MzA4O0FTOjEwNDEzMDM2NjQxMDc2NEAxNDAxODM4MDI1NTA2 https://www.researchgate.net/publication/7261460_Kim_JW_Tchernyshyov_I_Semenza_GL_Dang_CVHIF-1-mediated_expression_of_pyruvate_dehydrogenase_kinase_a_metabolic_switch_required_for_cellular_adaptation_to_hypoxia_Cell_Metab_3_177-185?el=1_x_8&enrichId=rgreq-e4392ea4-f659-4597-9cdf-54af3672b40b&enrichSource=Y292ZXJQYWdlOzI0NDM0MzA4O0FTOjEwNDEzMDM2NjQxMDc2NEAxNDAxODM4MDI1NTA2 https://www.researchgate.net/publication/7261460_Kim_JW_Tchernyshyov_I_Semenza_GL_Dang_CVHIF-1-mediated_expression_of_pyruvate_dehydrogenase_kinase_a_metabolic_switch_required_for_cellular_adaptation_to_hypoxia_Cell_Metab_3_177-185?el=1_x_8&enrichId=rgreq-e4392ea4-f659-4597-9cdf-54af3672b40b&enrichSource=Y292ZXJQYWdlOzI0NDM0MzA4O0FTOjEwNDEzMDM2NjQxMDc2NEAxNDAxODM4MDI1NTA2 https://www.researchgate.net/publication/7776528_Hypoxia-inducible_factor-1alpha_and_the_glycolytic_phenotype_in_tumors?el=1_x_8&enrichId=rgreq-e4392ea4-f659-4597-9cdf-54af3672b40b&enrichSource=Y292ZXJQYWdlOzI0NDM0MzA4O0FTOjEwNDEzMDM2NjQxMDc2NEAxNDAxODM4MDI1NTA2 strategies will better help to the understanding of the mo- lecular mechanisms underlying the metabolic and functional changes observed in cancer cells. Another transcription factor, the oncoprotein c-Myc also regulates the expression of GLUT1, HK, HPI, PFK-1, GAPDH, PGK, ENO, PYK, and LDH, thus, increasing glycolysis under aerobiosis [36–38]. This transcription factor also pro- motes mitochondrial biogenesis under nonhypoxic conditions [39]. The c-Myc oncogene is overexpressed in several tumors such as human LoVo colorectal tumor [40], glioblastoma multiforme [41], Burkitt’s lymphoma, prostatic intraepithelial neoplasias and prostatic carcinoma, melanoma, multiple my- eloma, breast carcinoma, and myeloid leukemia (reviewed in ref. 42). In primary breast cancer cells and Burkitt’s lym- phoma, a tight correlation between glycolytic rates and lev- els of c-Myc and HIF-1a is observed, suggesting crosstalk between the transcriptional factors [37,43]. 3. Glycolytic isoform expression and activity GLUT, HK, and PFK-1 are the main controlling steps of the glycolytic flux in erythrocytes, hepatocytes, and cardiac and skeletal muscle cells [44–47]. Changes in the isoform pattern of HK and PFK-1 expression occur in several tumor cells (Fig. 1) in comparison with normal cells (reviewed in ref. 2). As described later, it seems that such modifications in these and other glycolytic steps are part of the mechanisms involved in the increased glycolytic flux of tumor cells. Fig. 2. Mitochondrial metabolism in tumor cells. In glycolytic tumors: (1) Cytosolic pyruvate is transported into mitochondria through a deficient pyruvate transporter; (2) mitochondrial pyruvate is decarboxylated to acetoin which inhibits the tumor pyruvate dehydrogenase (PDH) complex; (3) truncated Krebs cycle with low aconitase and isocitrate dehydrogenase activities diminishes NADH pool; (4) increased citrate (Cit) efflux for cholesterol and fatty acids synthesis is developed; (5) lower expression of the respiratory chain complexes promotes a low H1 electrochemical gradient; (6) an increase in the inhibitory protein decreases the ATP synthase hydrolytic activity; (7) the close vicinity of HKII and ANT favors the direct transfer of mitochondrial ATP to HKII for glucose phosphorylation. In oxidative tumors: (8) Changes in the lipid composition of the inner mitochondrial membrane brings about a lower passive H1 permeability and a higher H1 gradient across the inner mitochondrial membrane; (9) a complete and fully functional Krebs cycle; (10) malate is transformed to pyruvate by an increased NADP1-dependent intramitochondrial malic enzyme; (11) glutamine (Gln) is actively oxidized by an over-expressed phosphate-activated glutaminase to form glutamate (Glut); (12) acetoacetate and b-hydroxibutyrate are actively oxidized to acetyl-CoA (AcCoA) by means of an increased succinyl-CoA acetoacetyl transferase (SCAAT); (13) a fraction of mitochondrial ATP is exported tothe cytosol to be used for cellular work. Abbreviations: Cit, citrate; OAA, oxaloacetate; Fum, fumarate; 2-Oxo, 2-oxoglutarate; RCC, respiratory chain complexes. [Color figure can be viewed in the online issue, which is available at www.interscience.wiley.com.] Energy metabolism of cancer cells 211 https://www.researchgate.net/publication/6055934_Hypoxia-Inducible_Factor_1_and_Deregulated_c-Myc_Cooperatively_Induce_Vascular_Endothelial_Growth_Factor_and_Metabolic_Switches_Hexokinase_2_and_Pyruvate_Dehydrogenase_Kinase_1?el=1_x_8&enrichId=rgreq-e4392ea4-f659-4597-9cdf-54af3672b40b&enrichSource=Y292ZXJQYWdlOzI0NDM0MzA4O0FTOjEwNDEzMDM2NjQxMDc2NEAxNDAxODM4MDI1NTA2 https://www.researchgate.net/publication/6055934_Hypoxia-Inducible_Factor_1_and_Deregulated_c-Myc_Cooperatively_Induce_Vascular_Endothelial_Growth_Factor_and_Metabolic_Switches_Hexokinase_2_and_Pyruvate_Dehydrogenase_Kinase_1?el=1_x_8&enrichId=rgreq-e4392ea4-f659-4597-9cdf-54af3672b40b&enrichSource=Y292ZXJQYWdlOzI0NDM0MzA4O0FTOjEwNDEzMDM2NjQxMDc2NEAxNDAxODM4MDI1NTA2 https://www.researchgate.net/publication/7756046_Myc_Stimulates_Nuclearly_Encoded_Mitochondrial_Genes_and_Mitochondrial_Biogenesis?el=1_x_8&enrichId=rgreq-e4392ea4-f659-4597-9cdf-54af3672b40b&enrichSource=Y292ZXJQYWdlOzI0NDM0MzA4O0FTOjEwNDEzMDM2NjQxMDc2NEAxNDAxODM4MDI1NTA2 https://www.researchgate.net/publication/5391511_c-Myc_overexpression_sensitises_colon_cancer_cells_to_camptothecin-induced_apoptosis?el=1_x_8&enrichId=rgreq-e4392ea4-f659-4597-9cdf-54af3672b40b&enrichSource=Y292ZXJQYWdlOzI0NDM0MzA4O0FTOjEwNDEzMDM2NjQxMDc2NEAxNDAxODM4MDI1NTA2 https://www.researchgate.net/publication/6436812_Metabolic_enzymes_regulated_by_the_Myc_oncogene_are_possible_targets_for_chemotherapy_or_chemoprevention?el=1_x_8&enrichId=rgreq-e4392ea4-f659-4597-9cdf-54af3672b40b&enrichSource=Y292ZXJQYWdlOzI0NDM0MzA4O0FTOjEwNDEzMDM2NjQxMDc2NEAxNDAxODM4MDI1NTA2 https://www.researchgate.net/publication/12493896_Deregulation_of_Glucose_Transporter_1_and_Glycolytic_Gene_Expression_by_c-Myc?el=1_x_8&enrichId=rgreq-e4392ea4-f659-4597-9cdf-54af3672b40b&enrichSource=Y292ZXJQYWdlOzI0NDM0MzA4O0FTOjEwNDEzMDM2NjQxMDc2NEAxNDAxODM4MDI1NTA2 https://www.researchgate.net/publication/10974673_Astroglial_c-Myc_Overexpression_Predisposes_Mice_to_Primary_Malignant_Gliomas?el=1_x_8&enrichId=rgreq-e4392ea4-f659-4597-9cdf-54af3672b40b&enrichSource=Y292ZXJQYWdlOzI0NDM0MzA4O0FTOjEwNDEzMDM2NjQxMDc2NEAxNDAxODM4MDI1NTA2 3.1. Glucose transporter In several tumor cells, the predominant overexpressed iso- form is GLUT1 (Table 1) [3,4]. However, other isoforms, which are not usually found in the tissue of origin, may also be overexpressed in some human leukemia, in kidney, lung, ovarian, and gastric cancers [4,5]. This de novo synthesis of GLUT might be part of the mechanisms promoting the increased glycolysis in tumor cells, because the GLUT activity also increases and significant control of the pathway resides in this step [10]; on the contrary, if this step does not exert control of glycolysis in some tumors, its increased level seems meaningless. In most studies on GLUT expression in human tumor cells (Barret, breast, cervical, colorectal, testicular carcino- mas, and glioblastoma), an enhanced mRNA or protein con- tent has been detected [4,48–50], but unfortunately GLUT ac- tivity was not determined. The GLUT1 Vmax is lower than the Vmax values of the glycolytic enzymes, suggesting that GLUT is the step with the higher control in glycolysis of rodent and human cancer cell lines. This finding emphasizes the relevance of developing new anti-GLUT target drugs, particu- larly for highly glycolytic-dependent tumors. 3.2. Hexokinase In tumor cells, HKII is the overexpressed isoform in the ma- jority of malignant cancer cells (Table 1), except for brain tumors in which HKI become the predominant isoform [51,52]. The HKII activity is 300–500 times higher in some rodent hepatomas than in rat liver cells, whereas in HeLa cells it is only seven times higher (reviewed in ref. 2, [10]). In mammalian normal cells, G6P is a potent inhibitor of HKI, HKII, and HKIII [51]. Also, the enhanced HK activity in tumor cells is counterbalanced by a strong G6P inhibition [10]. HK binding to mitochondria was proposed as a mecha- nism to circumvent the G6P blockade (reviewed in ref. 2). However, when assayed under near-physiological conditions of pH (7.0), temperature (37�C) and concentrations of glu- cose and G6P (>1 mM), the mitochondrial HK exhibits a sim- ilar sensitivity to G6P as its cytosolic counterpart in Table 1 Molecular mechanism involved in the enhanced glycolysis of human fast-growing tumors Human tumor type Ref. 1. Overexpression of selected HIF-1a glycolytic target enzymes and glucose transporters GLUT1 Bone (HOS), brain (Hs683, H4, A-172), breast (MDA-MB-231, MDA-MB-435, MCF-7, T47D), cervical (HeLa), choriocarcinoma (BeWo, JEG-3, JAr), colorectal (Caco-2, WiDr), epidermoid (A431), leukemia (K562, U937, HL60, Jurkat, H9), liver (HepG2), ovarian (A2780), pancreatic, renal (786-0), skin (HTB 63), squamous (UM-SCC22A, Scc-25) carcinomas [3–5] GLUT3 Breast (MDA-MB-231, T47D, ZR-75), choriocarcinoma (BeWo, JEG-3, JAr), Ischikawa en- dometrial cells, thyroid (papillary, follicular); lung, ovarian, and gastric carcinomas (biopsies) [4,6–8] HKI Colorectal (SW480, SW620) carcinoma [9] HKII Ependymoma, astrocitoma, glioma; pancreatic and cholangiocellular carcinoma (biopsies); cervical (HeLa), hepatocellular (HepG2) and alveolar (A549) carcinomas; stomach (AGS), and epidermoid (A431) cancers [10,11–13] PFK-L HL-60, KG-1, K-562 myeloid leukemia, MOLT-4 leukemia, lymphoma, HeLa and KB carcinoma, glioma [11,14] ALD-A and C, PGK-1, PGAM-B, ENO-a, LDHA Colorectal (SW480, SW620) carcinoma, hepatocellular carcinoma, squamous cell lung and pancreatic carcinomas and lung adenocarcinomas (biopsies) [15–18] 2. Low number of mitochondria or mitochondrial DNA content per cell Ovarian cancer, breast cancer, renal cell carcinoma [19,20] 3. Low expression and activity of OxPhos enzymes and transporters Krebs cycle enzymes Transformed mesenchymal cells, phaeochromocytomas, paragangliomas, liomyomas, leiomyosarcomas, renal cell, gastric and colon carcinomas, and papillary thyroid cancer [2,18,21–24] Respiratory complexes and ATP synthase Brain, mammary gland neoplasias; renal, squamous esophageal, lung, breast and gastric carcinomas. HeLa carcinoma; mammary tumors (Cf7, C3H); meningioma; ependymoma; pituitary adenoma; human kidney carcinoma 4. Increased mitochondrial DNA-sensitivity to reactive oxygen species Breast, colon, stomach, liver, kidney, bladder, head/neck and lung carcinomas; leukemia, and lymphoma. 25 212 BioFactors hepatocarcinoma AS-30D [10]. The presence of this G6P reg- ulatory mechanism of tumor HK supports the proposal of an essential role for this enzyme in the control of tumor glycol- ysis, despite its elevated overexpression [10]. This HK regu- lation mechanism has not been explored in other cancer cells, although it is expected to be present in those cells overexpressing HKI or HKII. Apparent specific inhibition of HK by 3-bromopyruvate (Fig. 3) was reported [53]. However, its cytotoxic activity against cancer cells was of low potency (IC90 ¼ 50–100 lM) [54]; and other glycolytic (GAPDH, PGK) and mitochondrial (PDH, SDH, glutamate dehydrogenase, pyruvate transporter) enzymes [53,55] are also sensitive to this compound, indicat- ing poor specificity. Clotrimazole (Fig. 3) induces HK detach- ment from mitochondria in B16 melanoma cells, but also detachment of PFK-1 and ALD from cytoskeleton in mouse LL/2 Lewis lung cancer and CT-26 colon adenocarcinoma, leading to diminished G6P, F1,6BP, and ATP levels, and gly- colytic flux (reviewed in ref. 56). Clotrimazole induces dimi- nution of cellular proliferation and viability in CT-26 colon carcinoma, Lewis lung carcinoma and breast cancer MCF-7 (IC50 ¼ 50–90 lM); and diminution of the size and develop- ment of intracranial gliomas (C6 and 9L), prolonging survival inrodents [56]. Lonidamine (Fig. 3) also blocks mitochondrial HK activity (65%) at lower doses (5–75 lM) than those used to induce tumor mortality in human fibrosarcoma (IC50 ¼ 150–500 lM) [56]. Although there are not specific HK inhibi- tors, some of the known HK inhibitors have been success- fully used in the cancer treatment by inducing increased sensitization to other anticancer drugs. 3.3. Phosphofructokinase-1 In different malignant tumors, PFK1-C, -L, or both, prevail over the M isoform (Table 1). On the other hand, overexpres- sion of both L and M isoforms are detected in human glio- mas, whereas in MOLT-4 leukemia, murine ascites and cervix carcinomas (HeLa, KB) the C isoform predominates [14,57]. PFK-1 from different sources shows variable kinetic properties depending on the isoform expressed and the tetra- meric complexes formed [58]. For example, PFK1-C from mu- rine ascites has a lower sensitivity to PEP, one of the physio- logical allosteric inhibitors of PFK-1, favoring an increase in the glycolytic flux [59]. Tumor PFK-1-M is less sensitive to in- hibition by ATP and citrate, and more sensitive to F2,6BP acti- vation, than normal PFK-1-C [60,61]. AMP activation of tumor PFK-1 is also enhanced, but this has not been further eval- uated probably because AMP seems ineffective to relieving the citrate and ATP inhibition (reviewed in refs. 2,10). Fig. 3. Anticancer drugs targeting glycolysis and OxPhos. Abbreviations: 3-BrPyr, 3-bromopyruvate; CTZ, clotrimazole; Goss, gossypol; IAA, iodoacetic acid; Rote, rotenone; Anti, antimycin; Cas IIgly, casiopeina-II glycine; cyanide-3- chlorophenylhydrazone, CCCP; Oligo, oligomycin; LCD, lipophilic cationic drugs; a-TOS, a-tocopherylsuccinate; DW, mitochondrial electrochemical gradient. [Color figure can be viewed in the online issue, which is available at www.interscience.wiley.com.] Energy metabolism of cancer cells 213 In several malignant rodent and human cells and established human tumor cell lines (Table 1), the PFK-1 activ- ity is 22–56 times higher than in non-tumorigenic cells [10,14]. In contrast, in human and rodent carcinomas (KB, thyroid) and brain tumors (gliomas, meningiomas, schwan- nomas, meduloblastoma), the PFK-1 activity is similar or even 1.3–2.5 times lower than its non-tumorigenic counter- part [14,61]. As the glycolytic flux is also enhanced in these other tumor cells, the decreased PFK-1 activity (i.e., content of active enzyme) suggests negligible control exerted by this step (6% in AS-30D glycolysis; [10]). These observations emphasize that not only changes on mRNA, protein content, or even enzyme activity, suffice to draw conclusions about how glycolysis changes in tumor cells. It is also necessary to analyze how the activity of key (e.g., controlling) pathway enzymes is regulated through changes in pathway intermedi- ary metabolites and modulator concentrations. 3.4. Lactate dehydrogenase A high LDH-A expression level correlates with aggressive forms of several different tumor types [62]. LDH-A knock- down in human breast cancer cells and LDH-A dowregulation in lymphoblastoid cells compromise their ability to prolifer- ate under hypoxia [63,64]. In addition, the tumorigenicity of the LDH-A-deficient cells is severely diminished and their respiration rate is increased by 50–60%; this phenotype is reversed by complementation with the human ortholog LDH-A protein [63]. Although it remains to be determined whether similar knockdown or downregulation of other gly- colytic steps also induces the same described phenotype, these studies show that the cancer energy metabolism can be a suitable therapeutic target. It was recently shown that lactate can be actively oxi- dized by aerobic tumor cells [65]. The authors proposed that, in solid tumors, lactate released from hypoxic cells may fuel the oxidative metabolism of the aerobic cellular subpopulation. For this lactate cycling, it is kinetically required that hypoxic cells express LDH-A and monocarboxy- late transporter 4 (MCT4), whereas aerobic cells should express LDH-B and MCT1; however, these aspects remain to be experimentally tested. 4. Evaluation of mitochondrial oxidative metabolism in cancer cells Warburg originally proposed that the driving force of the enhanced glycolysis in tumor cells was the energy deficiency caused by an irreversible damage of the mitochondrial func- tion [1]. There indeed seems to be a diminished oxidative metabolism in many tumor cell types. On this regard, some explanations have been advocated (Fig. 2), which, however, require to be critically reevaluated because several unsub- stantiated assumptions have been made. 4.1. Lower content of mitochondria per cell and deficient respiratory chain In 1978, Pedersen [66] proposed that the respiratory activity of isolated tumor mitochondria was as efficient as that of normal mitochondria, but that the diminished oxidative phosphorylation (OxPhos) observed in tumor cells was the result of a 20–50% lower content of mitochondria (Fig. 2; Ta- ble 1). This conclusion extended the original 1956 argument by Warburg [1] that the high glycolytic rate in tumor cells was due to a damaged respiratory chain (Fig. 2). Thus, a lower number of mitochondria per cell suggest that in tumor cells there are more active degradation mechanisms of mito- chondria (i.e., mitophagy; [67]) and/or a diminished de novo mitochondrial synthesis. These events have not been studied in tumors with a diminished number of mitochondria (Table 1). However, in von-Hippel-Lindau protein-deficient renal car- cinoma, HIF-1a expression diminishes mitochondrial biogene- sis and in consequence the cellular oxygen consumption [68]. In several carcinomas, HIF-1a is overexpressed suggest- ing that de novo mitochondrial synthesis may also be affected. Also, mitochondrial DNA diminishes during human ovarian and breast cancer progression and in highly aggres- sive tumors (renal cell carcinoma) [19,20,69], implying mitophagy activation. However, these results are in contradiction with other studies showing that the mitochondrial content of Morris 16 and 7800 hepatomas is similar to that of liver cells [66]; and that bronchial carcinoid and hepatoma mitochondria are abundant and exhibit normal morphology [66,70], although the mitochondrial functions were not determined. In Morris 7777 hepatoma similar COX, but lower succinase oxidase activity to those attained in rat liver mitochondria were described [71]. In a recent microarray analysis of the genes of the Krebs cycle enzymes it was found that citrate synthase, aco- nitase, isocitrate and succinate dehydrogenases, and fuma- rase, but not 2-oxoglutarate and malate dehydrogenases were downregulated in tumors while the opposite pattern was attained in transformed cells (Table 1) [21]. Furthermore, marked deficiencies have been identified in some mitochon- drial respiratory chain components from several human and rodent carcinomas (Table 1; Fig. 2) (reviewed in ref. 2). In contrast, an increase (2–5 times) in the activity of NADH cytochrome c reductase has also been determined in the same brain tumors and no differences in oxidative enzyme activities with normal cells have been detected for Morris and Novikoff hepatomas (reviewed in ref. 2) (Fig. 2). In mito- chondria isolated from some rat hepatomas, the ATP/ADP translocase activity was lower (5.4 times) than in normal liver mitochondria. In several human carcinomas, the ATP synthase was lower than in healthy human liver (Table 1) (reviewed in ref. 2, [22]). The tumor suppressor p53 activates TIGAR, a PFK-2 isoform that generates low F2,6BP levels, and hence unfa- vors glycolysis [72]. Moreover, p53 upregulates the COX sub- unit II protein expression [73], and down-regulates mRNA and protein expression of PGAM [74]. In cancer cells, p53 is 214 BioFactors often mutated, reduced, or deleted [75]. Some authors have proposed that this p53 inactivation provides a metabolic shift from respiratory to glycolytic metabolism although, in accordwith the TIGAR observations, it would rather favor mi- tochondrial oxidative metabolism [76]. Contradictory effects by the p53-modulated Erk and PI3K signaling pathways on the energy metabolism pathways awaits further experimen- tation to clearly establish the p53 role. It is pertinent to emphasize that diminution of one enzyme or transporter does not ensure a diminution in the pathway flux or metabolite concentration; the altered steps have to exert significant metabolic control, otherwise the alteration is silent. Unfortunately, the determination of the enzyme activities in tumor cells has not been always accom- panied by measurements of flux rate and steady-state metabolite concentrations. Likewise, detection of protein lev- els by western blot analysis or gene transcription by north- ern blotting or microarray analysis provides information with little functional meaning unless these measurements are accompanied by determination of activity and pathway flux. 4.2. Increased mitochondrial DNA (mtDNA) mutations and sensitivity to oxidative stress Thirteen protein components of the respiratory chain and ATP synthase are encoded by mtDNA. As mtDNA lacks histo- nes and there is lower capacity for DNA repair in normal mi- tochondria in comparison with the nuclear DNA (reviewed in ref. 2), it is thought that the enhanced oxidative stress in tu- mor cells induced by certain drugs may modify the normal transcription of mitochondrial genes (Table 1). Likewise, the higher frequency of somatic mtDNA mutations found in breast (61–74% of patients), bladder (51–100%), head and neck (51%), gastric (48%), colorectal (44–70%), brain (40%), hepatocellular (39–68%), thyroid (37–52%), lung (33–51%), ovarian (20%), prostate (11–19%), and other human cancers, might also presumably contribute to mitochondrial dysfunc- tion, although only a few mutations are known to have path- ological significance (reviewed in refs. 2,22). Surprisingly, 72% of the somatic mtDNA mutations found in cancer cells are also detected in the general healthy population [77] sug- gesting that most of these mutations are, simply, normal DNA duplication errors with no functional consequences. Germ-line mutations or downregulation of succinate dehydrogenase (SDH) and fumarate hydratase (FH) are asso- ciated with development of a variety of rather benign forms of phaeochromocytomas, paragangliomas, liomyomas, leio- myosarcomas, renal cell, gastric and colon carcinomas, and papillary thyroid cancer. These mutations inhibit SDH and FH activities, inducing succinate and fumarate accumulation and, hence, prolyl-hydroxylases inhibition, which in turn prompts an increased HIF-1a level (Table 1) (reviewed in ref. 78). These observations certainly suggest a diminished mito- chondrial function, but they do not demonstrate a complete blockade of the Krebs cycle flux or negligible respiratory or OxPhos rates. All these functions must be experimentally determined. 4.3. Lower Pyr oxidation; truncated Krebs cycle and lower reducing equivalents transfer These proposals were previously reviewed and analyzed [2]. No new information on this regard has been published, but recently it was demonstrated that prostate PC3 cancer accu- mulates high Zn2þ levels in mitochondria and cytosol. Zinc may inhibit aconitase, ‘‘truncating’’ the Krebs cycle flux (Fig. 2) and diminishing the reducing equivalent pool and cellular oxygen consumption [79]; however, by adding glutamine to the PC3 culture, the intracellular ATP level is restored, over- coming the aconitase inhibition by Zn2þ [80]. Therefore, the available data on the proposed deficiency of cancer cells in transfer equivalents from cytosol to mitochondria, acetoin inhibition and truncated Krebs cycle do not unequivocally establish a lower mitochondrial function in tumor cells. Furthermore, significantly marked differences should be found in the mechanism proposed for decreasing OxPhos in several tumors, not only in a selected one or two tumor types. Because of the genetic heterogeneity among the dif- ferent tumor cell types, it should not be expected a similar degree of modification in the mechanism proposed, but at least it should be observed in several tumor cell lines. In conclusion, there are tumor cell lines that certainly exhibit a decreased mitochondrial function, but that observa- tion does not seem to apply to all tumor cell types. There- fore, due to the genetic heterogeneity of tumor cells, OxPhos capacity should be experimentally evaluated for each particular tumor, to assess whether the enhanced gly- colysis is indeed accompanied by a significant depressed mitochondrial function. This last statement widely spread in the field (reviewed in refs. 2,76,81), has been taking as an established fact for tumor cell metabolism for many years, but because of the absence of hard experimental data it has rather become the metabolic central dogma of cancer. 5. Is oxidative phosphorylation damaged in most cancer cells? According to the Warburg hypothesis, the main oxidizable substrates in cancer cells should be hexoses such as glu- cose, fructose, and mannose; in turn, substrates oxidized by mitochondria should not be metabolized by cancer cells. In consequence, the main and only pathway providing ATP in cancer cells should be glycolysis; thus, negligible respiratory rates and insensitivity to mitochondrial inhibitors should also be expected. These assumptions are critically analyzed in the following sections. 5.1. Substrate utilization It is well-established that glucose is one of the carbon sour- ces preferentially consumed by fast-growth tumor cells (Fig. 1), together with glutamine, an exclusive mitochondrial oxi- dizable substrate (Fig. 2) (reviewed in ref. 2). In glycolytic tumors, an increased oxidation of glutamine is also observed. For the fast growing human cervix (HeLa), breast (MCF-7), prostate (PC3), colorectal (HT29) carcinomas, and Energy metabolism of cancer cells 215 slow-growing adenoma-derived cell line AA/C1, the ATP demand is supported by the aerobic oxidation of both glu- cose and glutamine [80,82–84], which indicates that glycoly- sis and OxPhos are both essential for ATP supply in these human tumor cells. A fully functional Krebs cycle able to supply NADH for OxPhos operates in AS-30D hepatoma (reviewed in ref. 2), and in PC3 carcinoma, in which aconitase activity is restored to the same level than that found in nontumorigenic tissues, when Zn2þ is removed [85]. In Caco-2 and Hep-G2 carcino- mas, several di and tricarboxilic transporters are upregulated to supply, continuosly, mitochondrial substrates for ATP pro- duction (Fig. 2) [86,87]. Mitochondrial tumor NADPþ-depend- ent malic enzyme is 10–20 times more active in tumor cells than in its origin tissue counterpart, thus, supplying NADH for the respiratory chain and pyruvate for LDH (Fig. 2). More- over, other oxidative pathways such as those for glutamine, glutamate, and ketone bodies are also highly active in tumor cells (Fig. 2) (reviewed in ref. 2). Cytosolic glutamine is transported faster (4–10 times) into tumor mitochondria and further transformed to glutamate by a strongly Pi-activated glutaminase with also higher activity (10–20 times versus normal liver mitochondria) (reviewed in ref. 2) (Fig. 2). Gluta- mine oxidation requires several Kreb cycle enzymes starting at 2-OGDH. Glutamine oxidation is the major anaplerotic pathway in gliomas and it is stimulated by estrogen in breast cancer; in addition, some c-Myc-transformed cells have an absolute requirement for glutamine in order to maintain viability through the continuous replenishment of Krebs cycle intermediates [88]. These observations suggest that glutamine oxidation is essential for tumor cell metabolism. The succinyl-CoA acetoacetyl transferase (SCAAT), enzyme that initiates ketone bodies oxidation, is 40-fold more active in AS-30D cells than in hepatocytes (reviewed in ref. 2) (Fig. 2). On the contrary, many brain tumors have lower SCAAT activity than normal neuronsand glia and, hence, are unable to metabolize ketone bodies. Then, as fatty acids do not pass the blood brain barrier, brain tumors seem to depend only on glucose, glycolysis and perhaps OxPhos for ATP supply (reviewed in ref. 2). In addition, dur- ing tumor cell proliferation, growth-factor signaling inhibits fatty acid b-oxidation, and stimulates lipid synthesis [88]. These accumulating evidences suggest an active mitochon- drial-dependent energy metabolism and a fully functional Krebs cycle in some tumor cell lines. 5.2. Oxygen concentration in tumors OxPhos is apparently limited by the low O2 availability inside the tumor [89]. Indeed, the prevalence of hypoxic areas (pO2 < 10 mm Hg; 14 lM; >50% of total tissue heterogeneously distributed) is characteristic of a wide variety of locally advanced human solid tumors [90]. In these hypoxic regions of human tumors as well as in the center of glioma and car- cinoma multicellular spheroids (a model that simulates the avascular stages of solid tumors), the determined O2 con- centration ranges from 1 to 61 lM [89,91,92], which resem- bles the range of values usually found in several normal tis- sues with normal blood irrigation (femoral muscle, mammary gland tissue) [93] (Table 2). However, OxPhos can only be compromised at O2 con- centration values lower than 1 lM because KmO2 of COX is 0.1–0.8 lM in different biological systems including ascites tumor cells [102–105]. In consequence, a saturating O2 con- centration for COX, and OxPhos, would be >4–8 lM (i.e., a substrate concentration of 10 times its Km value). Therefore, tumor mitochondrial metabolism would not be affected, in principle, by the hypoxia level found in tumors. On the other hand, prolonged exposure (weeks or months) to such hypoxic microenvironment indeed alters the expression of normal and tumor mitochondrial enzymes. Although the molecular mechanisms are still not clear, it has been proposed that HIF-1a or p53 are involved [73]. In fact, it has been described that a lengthy exposure (16–72 h) to hypoxia (1–20 lM O2) in HepG2 carcinoma and PC12 pheo- chromocytoma diminishes the mRNA level of mitochondrial enzymes (NADH dehydrogenase, COX, ATPase, glutaminase) Table 2 Oxygen concentration in human tumors Tumor type Organism O2 (lM) Ref. Head and neck squamous carcinoma Human 1 [94] Mammary adenocarcinoma Rat 3.5–42 [95,96] Cervix carcinoma Rat 7–29 [97] Mammary squamous carcinoma, lung and medulla Human <7 [98] Prostatic carcinoma Rat 2.0–9.1a [92,99] 11–112b Dunning Prostatic carcinoma Rat 14–61 [100,101] Fibrosarcoma Rat 15 [101] a Oxygen concentration determined in the center of solid tumor. b Oxygen concentration determined in the periphery of solid tumor. For other tumors, the oxygen concentration reported did not specify region. 216 BioFactors [106,107]. Unfortunately in these studies, the enzyme activ- ities and changes in hypoxia-associated transcription factors (HIF-1a and p53) were not evaluated. 5.3. Contribution of glycolysis and OxPhos to ATP supply It is intriguing that despite the accelerated glycolysis in sev- eral tumor cells, its total contribution to the cellular ATP supply only reaches 10% (reviewed in ref. 2) (Table 3). In marked contrast, in other tumor cell lines (Table 3), glycoly- sis indeed supports 50–70% of the ATP demand, a contribu- tion value also estimated by Warburg [1]. Moreover, the con- tribution of glycolysis and OxPhos to the ATP demand during the proliferative phase was similar in tumor cells with defi- cient oxidative system (Ehrlich hepatocarcinoma) (Table 3) [108]. To emphasize that OxPhos is a more efficient pathway than glycolysis to generate ATP, it is usually described that ‘‘OxPhos generates 36 or 38 ATP molecules per glucose, whereas glycolysis only generates 2 ATP molecules per glu- cose.’’ However, not all glucose, metabolized through the glycolytic pathway, actually generates lactate molecules, because a fraction of glucose may be drained to the branch- ing reactions. Thus, it is more accurate to determine the rate of lactate (þpyruvate) production as the more adequate pa- rameter of glycolytic ATP synthesis (1 lactate ¼ 1 ATP), and correcting for lactate formed from other sources (i.e., gluta- minolysis) with glycolytic inhibitors such as 2-deoxyglucose (2DOG). The rate of O2 consumption, sensitive to oligomycin, a specific ATP synthase inhibitor (Fig. 3), is the most adequate measurement of OxPhos, which is converted to rate of ATP synthesis by using the experimentally deter- mined P/O ratio of 2.5 for NADH and 1.5 for FADH2 in hepa- toma isolated mitochondria [110]. Thus, 30–32 ATP molecules generated per glucose fully oxidized is a more accurate value for OxPhos. There are few reports where metabolic control analysis (MCA) of the tumor energy metabolism has been experimen- tally carried out. MCA allows the quantification of the degree of control that an enzyme, pathway segment or entire path- way has on a particular pathway flux, metabolite concentra- tion, or cellular process [111,112]. By applying elasticity anal- ysis (an experimental approach of MCA) to glycolysis in AS- 30D tumor cells, it was found that the main flux-control (71%) resided in the first two pathway steps, that is, GLUT and HK [10]. The rest of the control (29%) was localized in the ALD-LDH segment, with a negligible contribution by PFK- 1 (<6 %). It was shown that, despite a remarkable overex- pression, tumor HK was strongly inhibited by its product G6P, thus, still being limiting for the pathway flux. On the other hand, PFK-1 was moderately overexpressed, but the tumor isoform was highly activated by F2,6BP, thus, surpass- ing the citrate and ATP inhibition. These findings provided a mechanistic explanation for the respective high and low flux control exerted by HK and PFK-1 (see Fig. 1). This study also showed that a massive over-expression of glycolytic enzymes does not lead to uncontrolled flux, but rather strict regula- tory mechanisms are preserved in tumor cells. Kinetic modeling of glycolysis in AS-30D and HeLa tu- mor cells has revealed that indeed GLUT and HK are the main flux-controlling steps in both tumors; and that HPI, inhibited by erythrose 4-phosphate and F1,6BP, modulates the supply of G6P towards pentose phosphate and glycogen synthesis pathways (Fig. 1) (A. Marı́n-Hernández, R. Moreno- Sánchez, and E. Saavedra, manuscript in preparation). Flux control analysis of the ATP synthesis in AS-30D hepatoma cells showed that OxPhos controlled by 66% whereas the ATP-consuming processes (protein and nucleic acid synthesis; ion ATPases) controlled by 34%. The main controlling step within OxPhos was the respiratory chain site Table 3 Energy metabolism in malignant tumor cells Tumor Organism Prevailing energy pathway % ATP contribution Glioma C6 Rat OxPhos 80 Oligodendroglioma, meningioma, medulloblastoma Human Glycolysis 60 Glioblastoma multiforme, Astrocytoma C6 Human, Rat Glycolysis and OxPhos 50 Transformed brain Hamster OxPhos 71 Colon sarcoma Human OxPhos 70 Novikoff hepatoma Rat Glycolysis 75 Ehrlich Lettré, Ehrlich, Walker-256, Morris 3683 and Dunings LC18 hepatomas; ascites mouse cancer; sarcoma 27 Rat, mouse Glycolysis and OxPhos 50 Reuber H-35, Morris (7793,7795, 7800, 5123), and AS-30D hepatomas Rat OxPhos 97 Lung carcinoma Human OxPhos 95 Breast cancer Human OxPhos 95 MCF7 breast carcinoma Human OxPhos 80 Melanoma Human OxPhos 97 HeLa cervix, ovarian and uterus carcinomas Human OxPhos 90 Modified from [2]. Energy metabolism of cancer cells 217 1 [113]. Control analysis of the tumor energy metabolism, ei- ther by establishing the main sites of control in glycolysis and OxPhos and/or by assessing the predominant energy pathway, may provide a more rational and quantitive approach for the identification and design of more specific therapeutic strategies whether the tumor cells are either of the glycolytic or the oxidative type. Therefore, it would be highly informative to carry out this kind of analysis with manyother different cancer models. 5.4. Mitochondrial inhibitors and respiration rates in tumor cells Some human and rodent gliomas exhibit high or moderate susceptibility to highly specific respiratory inhibitors; in addition, gliomas with glycolytic phenotype actively oxidize pyruvate and glutamine under low glucose [114]. These observations indicate the presence of fully functional mito- chondria and dependency on OxPhos. Oligomycin (Fig. 3) at low doses (0.06–0.7 lM), which do not affect normal cells, arrests the cell cycle progression from G1 to S phase in human promyelocytic leukemia (HL-60), and Jurkat T cells, due to a severe diminution of mitochondrial ATP production (reviewed in ref. 56). At 3–6 lM oligomycin, more than 50% of HL-60 cells are arrested in G2/M phase; however, this drug concentration may also affect normal cells. The respira- tory chain site 1 inhibitor rotenone (0.1–1 lM) (Fig. 3) arrests the cell cycle at G2/M promoting a strong inhibition (50– 90%) of cell proliferation in human lymphoma WP and 134 B osteosarcoma (reviewed in ref. 56). Rotenone inhibits respi- ratory chain site 1 (Fig. 3) in normal cells, but this drug might still be advantageously used for tumor cells as long as site 1 exerts a significantly higher flux control of OxPhos in tumor cells than in normal cells. Antimycin (IC50 ¼ 50 lM) (Fig. 3) diminishes proliferation by increasing ROS and hence apoptosis, loss of mitochondrial membrane potential, Bcl-2 down-regulation and Bax up-regulation in HeLa cells, by increasing ROS [115]. Classical uncouplers of OxPhos (Fig. 3) such as CCCP inhibit the growth of several malignant mam- mary carcinomas (EMT-6, M6H-U1). The action of this iono- phore consists in the acidification of the mitochondrial ma- trix, and collapse of the mitochondrial electrochemical Hþ gradient, which results in significant decrease of cellular ATP levels [116]. As originally claimed by Weinhouse [117], a wide vari- ety of tumor cell lines exhibit elevated rates of respiration (reviewed in refs. 2,56,109); whether this activity is fully associated with OxPhos remains to be determined (i.e., sen- sitivity to oligomycin). In AS-30D and HeLa monolayer cell cultures [83] and HeLa microspheroids [118], the rate of res- piration is 85–90% sensitive to oligomycin, indicating that the remaining 10–15% of the cellular O2 consumption was not associated to OxPhos. In tumor cells, the non-mitochon- drial oxygen-consuming enzymes, heme oxygenase and cyto- chrome P450 may also be overexpressed [119]; thus, the oxy- gen consumption values determined in the absence of oligomycin overestimate the rate of OxPhos. Therefore, the generalized statement that glycolysis predominates over OxPhos for ATP supply in tumor cells (reviewed in refs. 2,76,81) should be re-evaluated and exper- imentally determined for each particular type of tumor cell. An energy deficiency caused by a deteriorated OxPhos might indeed be the driving force behind the enhanced glycolysis in hypoxic tumors (in a process mediated perhaps by HIF-1a or p53), but a mitochondrial impairment does not seem to apply in nonhypoxic, oxidative tumors. Thus, the main ther- modynamic reason for increasing glycolysis in tumor cells (associated with either a damaged or an unaltered OxPhos) might rather be an energy deficiency induced by highly ATP- demanding processes such as an accelerated cellular prolif- eration and exacerbated nucleic acid, protein, and choles- terol synthesis. 6. Energy metabolism in tumor cells as therapeutic target A proportional relationship between the rate of cellular pro- liferation and the rate of ATP supply has been established for human (erythroleukemia K 562) and rodent (Ehrlich mouse carcinoma) fast-growth tumor cells [120,121]. How- ever, there is some discrepancy regarding the correlation between the degree of malignancy and the rate of ATP syn- thesis from glycolysis or OxPhos. Some authors have pro- posed that the glycolytic activity correlates with the degree of tumor malignancy, so that glycolysis is faster and OxPhos is slower in highly de-differentiated and fast-growing tumors than in slow-growing tumors or normal cells [66,122]. In fact, a high level of lactate has been proposed as a predictor of malignancy [123]. High serum LDH levels predict a poor out- come in pancreatic, lung, renal and testicular carcinomas, osteosarcoma, and melanoma. For human lung, colorectal, ovarian, larynx, breast, and hepatocellular carcinomas, high levels of GLUT1 or GLUT3, ALD-B, and HKII have been used as indicators of unfavorable prognosis [124,125]. There is a direct correlation between the tumor progression and the HK [10,52] and PFK-1 [10,59] activities. A high intracellular LDH-A (LDH-5) level correlates with a high serum level and with aggressive forms of several tumor types [62]. However, these correlations rely largely on nuclear LDH-5 expression. As localization of this glycolytic enzyme in the nucleus is atypical, the functional relevance of this expression pattern requires further experimentation [90]. Accordingly, it has been postulated that tumor cells that exhibit deficiencies in their oxidative capacity are more malignant than those that have an active OxPhos [126]. Fur- thermore, it seems that mtDNA mutations confer resistance to anticancer drugs. For instance, mutant mtDNA cybrids are more resistance to apoptosis and cisplatin than wild-type cells, and rho cells are extremely resistant to radiation, as well as to adriamycin, cisplatin, and etoposide [22,127]. Prostate cancer mutant (T8993G) cybrids (with an ATPase mutation) generated seven times larger tumors in nude mice than wild-type cybrids; this mutation causes impaired mito- chondrial ATPase synthesis [22]. 218 BioFactors 6.1. Energy metabolism anticancer drugs Certainly, drug efficacy, delivery, and side effects are prob- lems to be solved in developing new chemotherapies. In solid tumors, delivery to a hypoxic region may be difficult whether the drug does not easily permeate through the different cellular layers or whether drug expelling systems (i.e., P-glycoprotein, an organic anion ATPase that efficiently expels xenobiotics) are overexpressed [128]. To overcome these uncertainties, further searching and design of new specific drugs (i.e., molecules with inhibition constants in, at least, the submicromolar range and with superior membrane permeability) is required. Another problem associated with chemotherapy is that in many tumor types there is either inherent or acquired re- sistance to antineoplastic drugs. A significant advance has been the elucidation of the metabolic changes developed by the tumor cells for drug resistance. The drug-resistant cells decrease the mitochondrial Hþ electrochemical gradient by overexpressing the uncoupler protein 2 (UCP-2), which acts as a mitochondrial Hþ channel, collapsing the Hþ gradient generated by the respiratory chain. These cells also increase the utilization of alternative oxidizable substrates (fatty acids) [129]. Furthermore, drug-resistant tumor cells may also overexpress the P-glycoprotein to expel drugs such as doxorubicin, paclitaxel, vinblastine, and epirubicin [35]. Therefore, more selective targeting is required for the treat- ment of cancer. The observations of the previous section suggest that the blocking of glycolysis should arrest tumor progression. Indeed, inhibition of tumor glycolysis with 2DOG, 3-bromo- pyruvate, or lonidamide increases the sensitivity towards anticancer drugs commonly used in chemo-therapy such as cisplatin, 4-hydroperoxycyclophosphamide, melphalan, car- mustine, 1-b-D-arabinofuranosylcytocine, vincristine, taxol, adriamycin, etoposide, and camptothecin (reviewed in ref. 56). However, glycolytic inhibitors display low efficacy in arresting tumor growth, when used alone, which is also usu- ally accompanied by severe side effects in the host (reviewed in ref. 56). Muller et al. [108] originally proposed that a biochemi- cal strategy to efficiently suppress the acceleratedEhrlich mouse hepatoma proliferation was the simultaneous block- ade of both ATP-generating pathways. It appears difficult to target the energy metabolism of tumors as also the host cells depend on the same essential pathways for ATP supply. However, by identifying the most significant differences in the energy metabolism between tumor cells versus host cells, it might be possible to detect suitable antineoplastic targets (Figs. 1–3). It is worth noting that drugs used for in- hibiting OxPhos in cancer cells are not the classical specific and potent inhibitors such as rotenone, antimycin, oligomy- cin, and carboxyatractyloside, because they block the path- way in both malignant and healthy cells. Instead, these drugs are designed to be mitochondrially targeted only for cancer cells in virtue of their delocalized positive charge. Interestingly, the lipophilic cationic drugs rhodamines 6G and 123, and casiopeina-IIgly at low micromolar concentra- tions drastically abolish OxPhos and cell proliferation of Walker and AS-30D hepatomas, whereas glycolytic drugs such as gossypol, arsenite, and iodoacetate are ineffective (reviewed in ref. 56). Lipophilic cationic drugs (LCD) (Fig. 3) are accumulated in cytosol and mitochondria of tumor and normal cells because the elevated electrical potential gradient (Dw, nega- tive inside) generated across both the plasma membrane and inner mitochondrial membrane (reviewed in ref. 56). However, it is documented that mitochondria from human colon CX-1 tumor; cells and mitochondria from MCF-7 breast adenocarcinoma; neu-, v-Va-ras-, b-catenin, and c-myc-initi- ated mouse tumor cell lines; and A549 (nonsmall cell lung cancer), and glioblastoma M059K cells, develop a Dw of a higher magnitude (15–50 mV) than that of normal cells (epi- thelial cells from spleen, breast, kidney, small airway epithe- lial cells, fibroblasts, and pulmonary artery smooth muscle cells) (reviewed in refs. 35,56). Therefore, a significant higher lipophilic cation drug accumulation is achieved in tu- mor mitochondria. However, further studies on side effects of the lipophilic cations are required as the rhodocyanine MKT-077 showed severe nephrotoxicity in phase I trial and was discontinued [130]. The reasons for the higher Dw in tumor mitochondria might be related to the higher content of cardiolipin (increasing the density of membrane negative charges) and cholesterol (which may decrease the Hþ and other ions pas- sive diffusion) in the plasma and inner mitochondrial mem- branes [66,131]. In rho osteosarcoma cells, 50 times more rhodamine 123 is required to inhibit proliferation [132]. Recently, it was determined that the vitamin E ana- logue a-tocopheryl succinate (a-TOS) may specifically target (and freely diffuse) tumor cells by virtue of the more acidic extra and intracellular pH. Once inside the cell, a-TOS indu- ces apoptosis in mesothelioma and other tumors, without affecting normal cells, by apparently promoting an increased oxidative stress through the selective inhibition of SDH (Fig. 3) [133]. We recently reported that the growth of HeLa cells in multicellular spheroids involves changes in their energy metabolism in comparison with their counterpart in mono- layer culture [118]. In the spheroid initial formation, mito- chondria support more than 80% of the cellular ATP sup- ply. However, at later spheroid stages, mitochondrial metabolism fails and glycolysis becomes predominant. In this mature stage, tumor spheroids become highly sensi- tive to glycolytic inhibitors (2DOG, gossypol) [118]. Inter- estingly, casiopeina II-gly and rhodamine 123, laherradurin (an acetogenin extracted from Annonaceae plants that potently inhibits respiratory chain site 1) [118], and a-TOS block the initial cell cluster formation and growth of HeLa spheroids by directly inhibiting OxPhos (S. Rodrı́guez-Enrı́- quez, unpublished data). In multispheroids of human U118MG colon cancer, changing the prevalent metabolism from glycolytic to oxidative, by adding oxamate a LDH in- hibitor provokes an increase in the tumor sensitivity to radiation [91]. Energy metabolism of cancer cells 219 7. Tumor cell metabolism and positron emission tomography (PET) In recent years, PET combined with computed tomography (CT) has been applied for diagnosis, monitoring and treat- ment of cancer. PET has mainly used 18fluoro-deoxyglucose (FDG) as tracer under the assumption that tumors have a higher glycolytic capacity than normal cells (reviewed in ref. 2). FDG is transported into the cells by the glucose trans- porter, and then phosphorylated to FDG-6-phosphate (FDG-6- P) by HK [134]. FDG-6-P cannot be isomerized by HPI due to the C-2 fluor and it is slowly expelled, dephosphorylated, by the action of glucose-6-phosphatase. In consequence, it is trapped and accumulated in the neoplastic (and in some nontumorigenic) cells. Thus, by using FDG/PET it has been found that the vast majority of metastatic tumors (>90%) are highly glycolytic, in other words, there is a strict correla- tion between glycolytic activity and FDG uptake; it has also allowed the accurate and earlier detection (>90%) of differ- ent types of cancer [135]. 7.1. Limitations of the FDG/PET scan (A) The accuracy of the FDG/PET scan depends on the tumor stage. The FDG/PET may identify pancreatic cancer in advance stage with high sensibility (>85%) and moderate specifity (>53%), whereas in patients with early tumor stages (small tumor size) the sensibility decreases [136]. (B) False positives of FDG/PET scan have been frequently reported in infectious diseases, inflammatory cells, fibrotic lesions and other diseases [137,138]. Moreover, tumors with low glycolytic activity [137], carcinoid tumors, and bronchioalveolar lung carcinoma [139], as well as aggressive B-cell non-Hodgkin’s lymphoma treated with rituximab [140], reveal false negative results on FDG/PET scan. Bladder and prostate tumors are FDG-avid cancers but PET scan does not provide a clear diagnosis of these neoplasias [141]. In hepatocellular carcinoma, highly dif- ferentiated cancer cells are FDG-negative and poorly dif- ferentiated cancer cells are FDG-positive [142]. (C) OxPhos dependent tumors are not identified. In thyroid carcinoma, FDG is not concentrated, despite administra- tion of high and repetitive doses [143], suggesting that the relevant energy pathway in thyroid carcinoma is not glycolysis. Although FDG-PET serves an important role in the follow-up of patients with thyroid cancer, accurate localization of FDG-positive tissues is often difficult. The normal brain cells have a high glucose uptake, whereas the uptake of FDG in most brain tumors is similar or lower than in the normal tissue. (D) Variable sensitivity in hypoxic regions. Accumulation of FDG in malignant tumors is related to regional hypoxia, but a poor correlation between hypoxia and FDG uptake may appear. Therefore, FDG/PET cannot reliably differen- tiate hypoxic (i.e., glycolytic) from normoxic tumors in fre- quently hypoxic (head and neck cancer and glioblastoma multiforme) and less frequently hypoxic tumors (breast cancers) [144]. For rectal carcinoma, there is not signifi- cant difference in FDG uptake between patients with hypoxic tumors and those with normoxic tumors [145]. Knowing that not all tumors are glycolytic, but that some of them have a predominant oxidative metabolism or at least they have low glucose uptake (mediastinal lymph node, metastases of lung cancer, and prostate cancer) (see Table 3), it seems as a reasonable alternative to applying PET-CT with tracers directed to mitochondria. Copper (II)-pyruvaldehyde- bis (N4-methylthiosemicarbazone) (Cu-PTSM) was used for monitoring electron transport chain in normal brain mitochon- dria and Ehrlich ascites [146], and (60)Cu-diacetyl-bis (N(4)- methylthiosemicarbazone) ((60)Cu-ATSM) for detecting rectal carcinoma and uterine cervix cancer. Moreover, in prostate and hepatocellular carcinoma, the use of 11C-acetate/PET has been successfully validated byboth clinical and experimental studies [147], probably because the predominant energy pathway in these cancers is not glycolysis, but fatty acid oxi- dation, and hence, OxPhos [148]; 11C- and 18F-labeled choline analogues are also successful tracers for prostate cancer, he- patocellular carcinoma, and primary brain tumors. The use of mitochondrial tracers in PET analysis may en- counter the same difficulties described for FDG, regarding the detection of false negatives in low oxidative tumors, and false positives in normal tissues with high oxidative activity. The question of whether mitochondrial PET tracers may be more specific for tumors than for normal, healthy cells will be answered when more data become available, but it is worth noting that mitochondria of oxidative tumors develop a higher electrical membrane potential than mitochondria of normal tis- sue, thus favoring the accumulation of lipophilic, cationic drugs and facilitating the detection of oxidative tumors. 8. Conclusions All tumor cell types show an enhanced glycolytic flux; how- ever, not all of them have a diminished mitochondrial meta- bolic capacity. Therefore, not all tumor cell types depend exclusively on glycolysis for ATP supply; some of them may equally or predominantly rely on OxPhos (Table 3). We think that both energy pathways are not mutually excluding each other in cancer cells. In consequence, the driving force for the enhanced glycolysis in tumor cells cannot be an energy deficiency induced only by a damaged OxPhos. The acceler- ated cellular proliferation may also impose an energy defi- ciency (as well as a higher demand for glycolytic and Krebs cycle biosynthetic intermediaries), which can only be covered by an increased glycolysis, and an unperturbed OxPhos. Certainly, there is genetic, biochemical, and morpho- logical heterogeneity in cancer cells, but all of them do depend only on glycolysis and OxPhos for ATP supply. The enhanced tumor glycolysis results from an over-expression of most of the enzymes and transporters of the pathway, with HK and PFK-1 being markedly overexpressed in different isoforms (with different kinetic properties to that of the tis- sue of origin). At the genetic level, the enhanced glycolysis 220 BioFactors is primarily modulated by HIF-1a, although other transcrip- tion factors such as c-Myc and p53 may also been involved. These last two factors might also affect the mitochondrial function. In tumor types in which glycolysis is not the predomi- nant energy pathway, that is, in oxidative tumors (Fig. 2; Ta- ble 3), the application of mitochondria-directed drugs such as 11C-acetate or glutamine or 11C-rhodamines or casiopeinas in PET-CT analysis may be considered as alternative detec- tion and therapeutic strategies. These observations empha- size the necessity in advancing the understanding of tumor energy metabolism for improvement in diagnosis, drug design and chemotherapy of cancer. Traditional chemotherapy currently offers little long- term benefit for most malignant gliomas and is often associ- ated with adverse side effects that diminish the length or quality of life. Hence, new approaches are required that can provide long-term management of malignant brain tumors while permitting a better quality of life [149]. On this regard, it seems more rational for drug design to gather information by applying the metabolic control analysis, which allows the quantitative identification of the main controlling steps in a pathway, along with providing understanding of the underly- ing regulatory mechanisms and faciliting the prediction of the system behavior. The encouraging results with some energy-metabolism drugs indicate that, to successfully block growth of oxidative or partially oxidative tumors (Table 3), it is required to use simultaneously specific permeable drugs for glycolysis and OxPhos (reviewed in ref. 56). It may be argued that cancer cells are genetic and phenotypically heterogeneous from tu- mor to tumor. However, all tumor cell lines do depend on these two pathways for ATP supply. The metabolic therapy searches for physico- and biochemical differences between tumor and normal cells to improve the design of strategies that preferentially affect tumor metabolism and growth, without altering drastically the host tissue and organ func- tionality. This approach may complement the existent che- motherapeutic treatments, so that in combination may suc- cessfully stop tumor growth, invasiveness, and drug resistance. Acknowledgements The present work was partially supported by grants No. 80534 and 83084 from CONACYT-México. References [1] Warburg, O. (1956) On the origin of cancer cells. Science 123, 309–314. [2] Moreno-Sánchez, R., Rodrı́guez-Enrı́quez, S., Marı́n-Hernández, A., and Saavedra, E. (2007) Energy metabolism in tumor cells. FEBS J. 274, 1393–1418. [3] Reske, S. N., Grillenberger, K. G., Glatting, G., Port, M., Hildebrandt, M., Gansauge, F., and Beger, H. G. (1997) Overexpression of glucose transporter 1 and increased FDG uptake in pancreatic carcinoma. J. Nucl. Med. 38, 1344–1348. [4] Medina, R. A., and Owen, G. I. (2002) Glucose transporters: expres- sion, regulation and cancer. Biol. Res. 35, 9–26. [5] Noguchi, Y., Marat, D., Saito, A., Yoshikawa, T., Doi, C., Fukuzawa, K., Tsubaraya, A., Satoh, S., and Ito, T. (1999) Expression of facilitative glucose transporters in gastric tumors. Hepatogastroenterology 46, 2683–2689. [6] Medina, R. A., Meneses, A. M., Vera, J. C., Guzmán, C., Nualart, F., Rodrı́guez, F.De los Angeles Garcı́a, M., Kato, S., Espinoza, N., Monso, C., Carvajal, A., Pinto, M., and Owen, G. I. (2004) Differential regula- tion of glucose transporter expression by estrogen and progesterone in Ishikawa endometrial cancer cells. J. Endocrinol. 182, 467–478. [7] Ciampi, R., Vivaldi, A., Romeo, C., Del Guerra, A., Salvadori, P., Cosci, B., Pinchera, A., and Elisei, R. (2008) Expression analysis of facilitative glucose transporters (GLUTs) in human tyroid carcinoma call lines and primary tumors. Mol. Cell. Endocrinol. 291, 57–62. [8] Meneses, A. M., Medina, R. A., Kato, S., Pinto, M., Jaque, M. P., Liz- ama, I., de L. Garcı́a, M., Nualart, F., and Owen, G. I. (2008) Regula- tion of GLUT3 and glucose uptake by the cAMP signaling pathway in the breast cancer cell line ZR-75. J. Cell Physiol. 214, 110–116. [9] Yeh, C. S., Wang, J. Y., Chung, F. Y., Lee, S. C., Huang, M. Y., Kuo, C. W., Yang, M. L., and Lin, S. R. (2008) Significance of the glycolytic pathway and glycolysis related-genes in tumorigenesis of human col- orectal cancers. Oncol. Rep. 19, 81–91. [10] Marı́n-Hernández, A., Rodrı́guez-Enrı́quez, S., Vital-González, P. A., Flores-Rodrı́guez, F. L., Macias-Silva, M., Sosa-Garrocho, M., and Mor- eno-Sanchez, R. (2006) Determining and understanding the control of glycolysis in fast-growth tumor cells. Flux control by an over-expressed but strongly product-inhibited hexokinase. FEBS J. 273, 1975–1988. [11] Bennett, M. J., Timperley, W. R., Taylor, C. B., and Hill, A. S. (1978) Iso- enzymes of hexokinase in the developing, normal and neoplastic human brain. Eur. J. Cancer 14, 189–193. [12] Paudyal, B., Oriuchi, N., Paudyal, P., Higuchi, T., Nakajima, T., and Endo, K. (2008) Expression of glucose transporters and hexokinase II in cholangiocellular carcinoma compared using [18F]-2-fluoro-2-deoxy- D-glucose positron emission tomography. Cancer Sci. 99, 260–266. [13] Ong, L. C., Jin, Y., Song, I. C., Yu, S., Zhang, K., and Chow, P. K. (2008) 2-[(18)F]-2-Deoxy-D-Glucose (FDG) uptake in human tumor cells is related to the expresson of GLUT-1 and hexokinase II. Acta Radiol. 49, 1145–1153. [14] Vora, S., Halper, J. P., and Knowles, D. M. (1985) Alterations in the ac- tivity and isozymic profile of human phosphofructokinase durig malig- nant transformation in vivo and in vitro: Transformation-and progression-linked discriminants of malignancy. Cancer Res. 45, 2993–3001. [15] Ojika, T., Imaizumi, M., Abe, T.,and Kato, K. (1991) Immunochemical and immunohistochemical studies on three aldolase isozymes in human lung cancer. Cancer 67, 2153–2158. [16] Takashima, M., Kuramitsu, Y., Yokoyama, Y., Iizuka, N., Fujimoto, M., Nishisaka, T., Okita, K., Oka, M., and Nakamura, K. (2005) Overexpres- sion of alpha enolase in hepatitis C virus-related hepatocellular carci- noma: association with tumor progression as determined by proteomic analysis. Proteonomics 5, 1686–1692. [17] Chang, G. C., Liu, K. J., Hsieh, C. L., Hu, T. S., S.Charoenfuprasert, Liu, H. K., Luh, K. T., L.H.Hsu, C.W.Wu, Ting, C. C., Chen, C. Y., Chen, K. C., Yang, T. Y., Chou, T. Y., Wang, W. H., Whang-Peng, J., and Shih, N. Y. (2006) Identification of alpha-enolase as an autoantigen in lung can- cer: its overexpression is associated with clinical outcomes. Clin. Can- cer Res. 12, 5746–5754. [18] Mikuriya, K., Kuramitsu, Y., Ryozawa, S., Fujimoto, M., Mori, S., Oka, M., Hamano, K., Okita, K., Sakaida, I., and Nakamura, K. (2007) Expression of glycolytic enzymes is increased in pancreatic cancerous tissues as evidence by proteonomic profiling by two-dimensional elec- trophoresis. Int. J. Oncol. 30, 849–855. [19] Simmonet, H., Alazard, N., Pfeiffer, K., Gallou, C., C.Béroud, Demont, J., Bouvier, R., Schagger, H., and Godinot, C. (2002) Low mitochondrial respiratory chain content correlates with tumor aggressiveness in re- nal cell carcinoma. Carcinogenesis 23, 759–768. [20] Wang, Y., Liu, V. W., Xue, W. C., Cheung, A. N., and Ngan, H. Y. (2006) Association of decreased mitochondrial DNA content with ovarian can- cer progression. Br. J. Cancer 95, 1087–1091. Energy metabolism of cancer cells 221 [21] Funes, J., Quintero, M., Henderson, S., Martinez, D., Qureshi, U., West- wood, C., Clements, M. O., Bourboulia, D., Pedley, R. B., Moncada, S., and Boshoff, C. (2007) Transformation of human mesenchymal stem cells increases their dependency on oxidative phosphorylation for energy production. Proc. Natl. Acad. Sci. USA 104, 6223–6228. [22] Chatterjee, A., Mambo, E., and Sidransky, D. (2006) Mitochondrial DNA mutations in human cancer. Oncogene 25, 4663–4674. [23] Selak, M. A., Armour, S. M., MacKenzie, E. D., Boulahbel, H., Watson, D. G., Mansfield, K. D., Pan, Y., Simon, M. C., Thompson, C. B., and Gottlieb, E. (2005) Succinate links TCA cycle dysfunction to oncogene- sis by inhibiting HIF-alpha prolyl hydroxylase. Cancer Cell. 7, 77–85. [24] Pollard, P. J., Briere, J. J., Alam, N. A., Barwell, J., Barclay, E., Wortham, N. C., Hunt, T., Mitchell, M., Olpin, S., Moat, S. J., Hargreaves, I. P., Heales, S. J., Chung, Y. L., Griffiths, J. R., Dalgleish, A., MacGrath, J. A., Gleeson, M. J., Hodgson, S. V., Puolsom, R., Rustin, P., and Tomlin- son, I. P. (2005) Accumulation of Krebs cycle intermediates and over- expression of HIF1alpha in tumours which result from germline FH and SDH mutations. Hum. Mol. Genet. 14, 2231–2239. [25] Penta, J. S., Johnson, F. M., Wachsman, J. T., and Copeland, W.C. (2001) Mitochondrial DNA in human malignancy. Mutat. Res. 488, 119–133. [26] Stubbs, M., Bashford, C. L., and Griffiths, J. R. (2003) Understanding the tumor-metabolic phenotype in the genomic era. Curr. Mol. Med. 3, 49–59. [27] Balinsky, D., Platz, C. E., and Lewis, J. W. (1984) Enzyme activities in normal, dysplastic, and cancerous human breast tissues. J. Natl. Can- cer. Inst. 72, 217–224. [28] Walenta, S., and Mueller-Klieser, W. F. (2004) Lactate: mirror and motor of tumor malignancy. Semin. Radiat. Oncol. 14, 267–274. [29] Altenberg, B., and Greulich, K. O. (2004) Genes of glycolysis are ubiq- uitously overexpressed in 24 cancer classes. Genomics 84, 1014–1020. [30] Robey, I. F., Lien, A. D., Welsh, S. J., Baggett, B. K., and Gillie, R. J. (2005) Hypoxia-inducible factor-1a and the glycolytic phenotype in tumors. Neoplasia 7, 324–330. [31] Krieg, M., Haas, R., Brauch, H., Acker, T., Flamme, I., and Plate, K. H. (2000) Up-regulation of hypoxia-inducible factors HIF-1alpha and HIF- 2alpha under normoxic conditions in renal carcinoma cells by von Hip- pel-Lindau tumor suppressor gene loss of function. Oncogene 19, 5435–5443. [32] Papandreou, I., Cairns, R. A., Fontana, L., Lim, A. L., and Denko, N. C. (2006) HIF-1 mediates adaptation to hypoxia by actively downregulat- ing mitochondrial oxygen consumption. Cell. Metab. 3, 187–197. [33] Kim, J. W., Tchernyshyov, I., Semenza, G. L., and Dang, C. V. (2006) HIF-1-mediated expression of pyruvate dehydrogenase kinase: a meta- bolic switch required for cellular adaptation to hypoxia. Cell. Metab,3, 177–185. [34] McFate, T., Mohyeldin, A., Lu, H., Thakar, J., J.Henriques, Halim, N. D., Wu, H., Schell, M. J., Tsang, T. M., Teahan, O., Zhou, S., Califano, J. A., Jeoung, N. H., Harris, R. A., and Verma, A. (2008) Pyruvate dehydro- genase complex activity controls metabolic and malignant phenotype in cancer cells. J. Biol. Chem. 283, 22700–22708. [35] Bonnet, S., Archer, S. L., J.Allalunis-Turner, Haromy, A., Beaulieu, C., Thompson, R., Lee, C. T., Lopaschuk, G. D., Puttagunta, L., Bonnet, S., Harry, G., Hashimoto, K., Porter, C. J., Andrade, M. A., Thebaud, B., and Michelakis, E. D. (2007) A mitochondria-Kþ channel axis is sup- pressed in cancer and its normalization promotes apoptosis and inhib- its cancer growth. Cancer Cell. 11, 37–51. [36] Osthus, R. C., Shim, H., Kim, S., Li, Q., Reddy, R., Mukherjee, M., Xu, Y., Wonsey, D., Lee, L. A., and Dang, C. V. (2000) Deregulation of glu- cose transporter 1 and glycolytic gene expression by c-Myc. J. Biol. Chem. 29, 21797–21800. [37] Kim, J. W., Gao, P., Liu, Y. C., Semenza, G. L., and Dang, C. V. (2007) Hypoxia-inducible factor 1 and dysregulated c-Myc cooperatively induce vascular endothelial growth factor and metabolic switches hex- okinase 2 and pyruvate dehydrogenase kinase 1. Mol. Cell. Biol. 27, 7381–7391. [38] Rimpi, S., and Nilsson, J. A. (2007) Metabolic enzymes regulated by the Myc oncogene are possible targets for chemotherapy or chemo- prevention. Biochem. Soc. Trans. 35, 305–310. [39] Li, F., Wang, Y., Keller, K. I., Potter, J. J., Wonsey, D. R., O’Donnell, K. A., Kim, J. W., Yustein, J. T., Lee, L. A., and Dang, C. V. (2005) Myc stimulates nuclearly encoded mitochondrial genes and mitochondrial biogenesis. Mol. Cell. Biol. 25, 6225–6234. [40] Arango, D., Mariadson, J. M., Wilson, A. J., Yang, W., Corner, G. A., Nicholas, C., Aranes, M. J., and Augenlicht, L. H. (2003) c-Myc overex- pression sensitizes colon cancer cells to camptothecin-induced apo- ptosis. Br. J. Cancer 89, 1757–1765. [41] Jensen, N. A., Pedersen, K. M., Lihme, F., Rask, L., Nielsen, J. V., Ras- mussen, T. E., and Mitchelmore, C. (2003) Astroglial c-Myc overexpres- sion predisposes mice to primary malignant gliomas. J. Biol. Chem. 278, 8300–8308. [42] Nesbit, C. E., Tersak, J. M., and Prochownik, E. V. (1999) MYC onco- genes and human neoplastic diseases. Oncogene 18, 3004–3016. [43] Robey, I. F., Stephen, R. M., Brown, K. S., Baggett, B. K., Gatenby, R. A., and Gillies, R. J. (2008) Regulation of the Warburg effect in early- passage breast cancer cells. Mol. Cell. Biol. 27, 7381–7393. [44] Rapoport, T. A., Heinrich, R., and Rapoport, S. M. (1976) The regula- tory principles of glycolysis in erythrocytes in vivo and in vitro. A min- imal comprehensive model describing steady states, quasi-steady states and time-dependent processes. Biochem. J. 154, 449–469. [45] Torres, N. V., Mateo, F., Meléndez-Hevia, E., and Kacser, H. (1986) Kinetics of metabolic pathways. Biochem. J. 234, 169–174. [46] Torres, N. V., Souto, R., and Meléndez-Hevia, E. (1989) Study of flux and transition time control coefficient profiles in a metabolic system in vitro and the effect of an external stimulator. Biochem. J. 260, 763–769. [47] Kashiwaya, Y. K., Sato, K., Tsuchiya, N., Thomas, S., Fell, D. A., Veech, R. L., and Passonneau, J. V. (1994) Control of glucose utilization in working perfused rat heart. J. Biol. Chem. 269,
Compartilhar