Cancer Research Meeting Calendar Jordan
HOME HELP FEEDBACK SUBSCRIPTIONS ARCHIVE SEARCH TABLE OF CONTENTS
Cancer Research Clinical Cancer Research
Cancer Epidemiology Biomarkers & Prevention Molecular Cancer Therapeutics
Molecular Cancer Research Cancer Prevention Research
Cancer Prevention Journals Portal Cancer Reviews Online
Annual Meeting Education Book Meeting Abstracts Online
This Article
Right arrow Full Text (PDF)
Right arrow Alert me when this article is cited
Right arrow Alert me if a correction is posted
Services
Right arrow Email this article to a friend
Right arrow Similar articles in this journal
Right arrow Similar articles in PubMed
Right arrow Alert me to new issues of the journal
Right arrow Download to citation manager
Right arrow reprints & permissions
Citing Articles
Right arrow Citing Articles via HighWire
Right arrow Citing Articles via Google Scholar
Google Scholar
Right arrow Articles by Martin, D. S.
Right arrow Articles by Koutcher, J. A.
Right arrow Search for Related Content
PubMed
Right arrow PubMed Citation
Right arrow Articles by Martin, D. S.
Right arrow Articles by Koutcher, J. A.
[Cancer Research 60, 6776-6783, December 15, 2000]
© 2000 American Association for Cancer Research

Perspectives in Cancer Research

ATP Depletion + Pyrimidine Depletion Can Markedly Enhance Cancer Therapy: Fresh Insight for a New Approach1

Daniel S. Martin2, Joseph R. Bertino and Jason A. Koutcher

Memorial Sloan-Kettering Cancer Center, New York, New York 10021

Introduction

In the 1980s, necrosis was considered the mode of cell death induced by DNA-damaging anticancer agents because of the activity of PARP.3 PARP is activated by the DNA strand breaks caused by anticancer agents and cleaves the glycolytic coenzyme, NAD+, leading to formation of poly(ADP-ribose) moieties. The ensuing depletion of NAD+ inhibits glycolytic generation of ATP with consequent ATP depletion, eventuating in necrotic cell death (Fig. 1)Citation .



View larger version (16K):
[in this window]
[in a new window]
[Download PPT slide]
  		Fig. 1. DNA strand breaks activate PARP, which cleaves NAD into PAR moieties. The result is a marked decrease in NAD+ with a consequent fall in ATP until finally there is insufficient ATP to sustain survival of the cell, and cell death by necrosis occurs.

 
Heterogeneous neoplastic cell populations likely contain cancer cells of variable sensitivity to the anticancer agents. Less sensitive cells would not receive enough damage to reduce ATP to low levels sufficient to cause necrotic death. We hypothesized that biochemical modulation to further depress ATP to lower lethal-inducing levels would kill these sublethally injured cells, augment tumor regressions, and perhaps even yield some cures.

The ATP-Depleting and Pyrimidine-depleting Agents

Biochemical modulation is the manipulation of intracellular metabolic pathways by agents to produce selective enhancement of antitumor effects by the anticancer agent (1) . Because damage to the glycolytic generation of ATP in cancer cells was shown to occur after the administration of DNA-damaging anticancer agents (2, 3, 4, 5, 6, 7) , 6-AN, an NAD antagonist, known to inhibit glycolytic production of ATP (8, 9, 10, 11, 12, 13) , was administered with anticancer agents to further deplete intracellular ATP.

MMPR, known to inhibit de novo purine biosynthesis (14 , 15) and thereby limit adenine supplies for ATP production, was also concomitantly administered. In high dosage, MMPR also decreases pyrimidine ribonucleotide concentrations in vitro (16) . Because a de novo pyrimidine synthesis inhibitor, PALA, as a single agent in low nontoxic dosage can selectively lower pyrimidine nucleotide levels in tumors (17) , low-dose PALA was added to MMPR therapy to further lower the reduction of pyrimidine synthesis by MMPR. The three agents PALA, MMPR, and 6-AN were evaluated alone, in various double combinations, and as a triple combination against advanced breast tumors in mice. Pooled experiments (18 , 19) demonstrated that neither the maximum tolerated dose of MMPR alone, nor 6-AN alone, nor the double combination of PALA + 6-AN produced cell kill. There were no partial regressions of tumors (PR, >=50% tumor shrinkage in the volume of the initially measured tumor). However, tumor growth was inhibited in these groups as compared with saline controls.

Cell cycle events (i.e., proliferation) require a minimal ATP content to undergo proliferation. If ATP depletion is reduced to levels >15% of normal but is below the minimal level necessary for cell division, only proliferation arrest (i.e., tumor growth inhibition) and not cell death (i.e., tumor regression) will ensue (20 , 21) . Table 1Citation records that MMPR alone (group 1) and 6-AN alone (group 2) depress tumor ATP levels 48 h after treatment to 34 and 69%, respectively, compared with saline-treated control tumors. These are ATP levels compatible with the tumor growth inhibitions produced by MMPR alone and 6-AN alone in the above-pooled published experiments (18 , 19) . PALA does not effect ATP depletion and in the low dosage that was administered reduces pyrimidine biosynthesis but does not have anticancer activity (17) . Hence, the above-noted combination of low dose PALA + 6-AN only inhibited tumor growth attributable to the 6-AN, which alone only reduced ATP to 69% of normal (48 h, group 1; Table 1Citation ).


View this table:
[in this window]
[in a new window]

  		Table 1 Effect of MMPR + 6-AN + PALA on tumor ATP pools in CD8F1 micea

 
In contrast, the double combination of MMPR (a strong ATP depleter, 34% of normal, 48 h, group 1; Table 1Citation ) plus PALA (which is devoid of an ATP-depleting effect) produced a very few partial tumor regressions, 7% PR (18 , 19) . The MMPR-induced depletion of ATP to 34% is an average; hence, a few individual tumors likely have an ATP level <=15% of normal, a level shown to be insufficient to sustain cell viability (20 , 21) , and particularly in the presence of the severe pyrimidine depletion produced by the double combination of PALA + MMPR, as is explained below.

Please note that the murine tumors in these experiments are first-passage s.c. transplants from a tumor brei made by mixing the cancer cells of three or four single, spontaneous, autochthonous breast tumors, the CD8F1, tumor model included previously in the National Cancer Drug Screening Program (23, 24, 25) . All spontaneous tumors, whether human or murine, have a heterogeneous neoplastic cell population. Because each experiment consists of a brei composed of several different spontaneous tumors, the neoplastic cell composition is somewhat different form experiment to experiment, resulting in some quantitative differences between experiments. However, each experiment has its own control, and the results are quantitatively relevant within individual experiments, as are trends among experiments.

In this series of three pooled published experiments, the double combination of MMPR + 6-AN produced an objective response rate of 17% PR (18 , 19) . This therapeutic result is compatible with the MMPR + 6-AN-induced cell killing average ATP level of 15% of normal (Table 1Citation ; group 3, 48 h). Note that the low ATP level of 15% induced by MMPR + 6-AN is, as expected, unchanged (still 15%) by the addition of PALA to MMPR + 6-AN (group 4; Table 1Citation ). However, in the presence of this severe limitation to ATP availability (15% of normal), the triple drug combination of MMPR + 6-AN + PALA produced a PR rate of 61% (18 , 19) . The severely depleted ATP levels likely inhibit the salvage pathway formation of pyrimidine di- and triphosphates at the kinase step. Pyrimidine nucleotides serve essential functions in nucleic acid metabolism and sugar nucleotide formation for glycosylation of proteins and lipids. It is not surprising that severe inhibition of pyrimidine biosynthesis (because of PALA + high-dose MMPR), in the presence of severe ATP depletion (because of MMPR + 6-AN), enhances tumor regressions over MMPR + 6-AN (18 , 19) . The UTP pools in the in vivo MAP-treated tumors were sharply reduced to 14% of normal (18) . It is the severe lowering of ATP levels (15% of normal) that is the key ingredient that allows the severe pyrimidine depletion to appreciably augment the anticancer activity of MAP (a 61% PR) over that of MMPR + 6-AN (a 17% PR).

Although MMPR + 6-AN causes the all-important ATP depletion to cancer cell-killing levels of <=15% of normal (20 , 21) , another reason for including PALA with MMPR + 6-AN (i.e., MAP) is pertinent to the administration of DNA-damaging anticancer agents. The induction of apoptosis by the anticancer agents causes mitochondrial damage in sublethally injured cancer cells. Pyrimidine de novo synthesis is functionally linked to the respiratory chain in the inner mitochondrial membrane by mitochondrial-bound dihydrooratate dehydrogenase, the fourth enzyme of de novo pyrimidine synthesis. Thus, PALA (+ high-dose MMPR) should further lower the reduction of pyrimidine levels attributable to the mitochondrial damage effected by an anticancer agent-induced apoptotic biochemical cascade in surviving but sublethally injured cells. It has been shown previously that cells that had been completely depleted of mitochondria become pyrimidine auxotrophs because of the deficiency of the respiratory chain-dependent dihydrooratate dehydrogenase (26) . A minimal level of pyrimidine nucleotides is essential to sustain cell life. MAP severely reduces both ATP and pyrimidine levels in cancer cells. In cancer cells sublethally injured by anticancer agents, ATP and pyrimidine levels are depleted by the mitochondrial damage induced by the apoptotic biochemical cascade initiated by the anticancer agent. Anticancer agents produce a tumor regression rate by directly killing many cancer cells by either necrosis or apoptosis, but they also effect sublethal injury to less sensitive cancer cells from which they will recover. MAP targets their sublethally injured cancer cells before they can recover, further decreasing their ATP and pyrimidine levels, killing these cells, and thereby markedly enhancing tumor regressions. It is the anticancer agents that preferentially reduce ATP and pyrimidines, two metabolites that are essential for cell viability, to low levels in sublethally injured cancer cells, thereby creating a therapeutic opportunity for biochemical modulation (e.g., MAP) to further reduce them to lower levels insufficient to sustain the recovery of these injured cancer cells.

The central importance of severe ATP depletion to the tumor regressions (i.e., cancer cell deaths) produced by MAP is illustrated in our in vivo experiments published previously (27) investigating the prolonged retention (4 days) of intracellular MMPR-P after MAP administration to mice bearing advanced tumors. MMPR is phosphorylated by adenosine kinase to MMPR-P, which inhibits de novo purine synthesis at the level of amidophosphoribosyl transferase, and this inhibition causes ATP depletion. The MMPR depletion of ATP is driven by prolonged MMPR-P levels over an extended period (4–5 days) because of continuous resynthesis of MMPR-P by adenosine kinase. After MAP administration, tumor ATP measurements (% of control) on days 2, 3, 4, and 5 averaged 52, 38, 35, and 50%, respectively, and MMPR-P was retained in the tumors at a high level over this prolonged period. The average ATP measurements of 38 and 35% likely include cell-killing ATP values <=15% of normal because three partial tumor regressions were produced among 10 advanced tumor-bearing mice. Another group of 10 mice bearing the same transplants of advanced tumors received the same MAP treatment, followed 6 h later with iodotubercidin, an inhibitor of adenosine kinase, to allow an initial period of synthesis of MMPR-P prior to inhibition of adenosine kinase by iodotubercidin. However, this treatment prevented both the prolonged accumulation of MMPR-P and strong ATP depletion, producing tumor ATP values (% of control) of only 56, 53, 74, and 88% on days 2, 3, 4, and 5. In the presence of such poor ATP depletion, there were no partial tumor regressions.

The data (27) demonstrate that severe ATP depletion is necessary and central to MAP-induced tumor regression. Pyrimidine depletion (i.e., PALA) makes a substantial contribution to achieving still more cancer cell deaths (i.e., greater tumor regressions) only in the presence of severe ATP depletion. The biochemical damage done to sublethally injured cancer cells by anticancer agents renders these cells vulnerable to cell death by severe ATP-pyrimidine depletion.

ATP depletion clearly occurs, even without the ATP-depleting contribution of an apoptosis-inducing DNA-damaging anticancer agent (Fig. 1)Citation . The combination of only MMPR + 6-AN has been shown to effect severe lowering of tumor ATP levels in tumor-bearing animals. Specifically, the tumors of mice treated with MMPR + 6-AN (Group 3; Table 1Citation ) show a depletion to 15% of normal 48 h after administration (28) .

MAP + Radiotherapy

The MAP regimen, when combined with radiation, produced cures for the first time in the murine advanced spontaneous breast tumor system, demonstrating the potential for this new therapeutic approach to convert merely palliative (i.e., temporary tumor remission) treatment to curative therapy (29) . Cures are claimed because the advanced murine tumors (treated when the tumor-bearing mice were 3 months old with only three intermittent courses of MAP + radiation every 10–11 days ending at day 21) underwent complete tumor regressions, which continued in 25% of the mice for >1 year (380 days). In contrast, no complete regressions were obtained with MAP alone, and only one short-lived complete tumor regression was obtained in animals treated with radiation alone.

Summary of Preclinical Therapeutic Results with MAP + Cancer Chemotherapy

MAP plus each of eight mechanistically different anticancer drugs were administered to advanced tumor-bearing mice with a variety of tumor types (murine breast cancers, colon tumors, leukemia, and human breast cancer xenografts). The biochemical modulatory effort with MAP dramatically enhanced treatment of these tumors with agents that included doxorubicin, paclitaxel, cisplatin, 5-fluorouracil, phenylalanine mustard, cyclophosphamide, mitomycin C, and etoposide (29, 30, 31, 32, 33, 34, 35, 36) . The overall antitumor results with a variety of anticancer agents demonstrated safe and impressive significant augmentation of tumor regression, including complete regressions, and even some (25%) cures (29) .

The addition of MAP to combination chemotherapy with two anticancer agents (FU + Adr) was safe, without need for dose reduction, and yielded enhanced antitumor activity, including complete regressions not achieved previously (32) . The results encourage the prospect of the safe addition of MAP to a large number of anticancer agents in combination with the likelihood of even greater anticancer results (e.g., after increased complete regressions comes cures).

Preclinical MAP Toxicity

MAP can cause body weight loss in mice. However, this weight loss is not accompanied by diarrhea or by histopathological changes in organs (such as the intestine). A severe decrease in eating and drinking for 3–4 days after each of the three courses of intermittent chemotherapy was noted. Treatment-conditioned weight loss because of failure to eat or drink is not unusual for animals receiving intensive chemotherapy. Importantly, weight loss, which can indeed cause inhibition of tumor growth, does not produce tumor regression. The therapeutic activity measured in all of our studies used the stringent clinical criterion of tumor regression (i.e., 50% or greater decrease in tumor size). We have done separate experiments (unpublished) demonstrating that weight loss does not cause tumor regression. This fact is also clearly apparent in some of our published studies with ATP-depleting therapy. For example, in a pooled series of six experiments, two groups had similar weight loss (-17 and -19%), but one group had 60% tumor regressions and the other had only 2% tumor regressions. Also, in that same series of experiments, two other groups had identical weight loss (-25%) but different tumor regression rates (60% versus 79%) that were statistically significant. Weight loss would not be a problem in patients who, unlike animals, can be persuaded to drink and eat or can be supported i.v.

ATP Depletion in Tumors with MTAP Deficiency

MTAP, an enzyme involved in purine metabolism, is present in normal tissues but frequently is deleted (deficient) in leukemias, brain tumors, non-small cell lung cancers, breast cancers, melanomas, pancreatic cancers, and sarcomas (37, 38, 39, 40, 41, 42) .4 Methylthioadenosine is produced during polyamine synthesis and cleaved to adenine and 5-methylthioribose-1-phosphate by MTAP. The adenine is reconverted to AMP and then to ATP. The deletion of the MTAP gene in many tumors results in the inability of these cancer cells to salvage adenine; the ATP pools in these cells must be depleted. L-Alanosine, a potent inhibitor of de novo AMP synthesis has demonstrated selective anticancer activity in vitro in MTAP-negative cell lines as compared with MTAP- positive cell lines (42) .

An examination of MTAP expression in 10 human soft tissue sarcoma cell lines found MTAP not detectable in 3 of the 10 cell lines. These three cell lines were >10-fold more sensitive to L-alanosine than the cell lines containing MTAP. The addition of the de novo purine synthesis inhibitor, MMPR, further enhanced the sensitivity of the cells lacking MTAP activity to L-alanosine. These results provide the basis of selective therapy using L-alanosine + MMPR to treat patients with soft tissue sarcomas and are another example of the therapeutic utility of the ATP-depleting strategy. In vivo studies of L-alanosine + MMPR, as well as the addition of 6-AN, are being evaluated (43) .

Recognition of Apoptosis as the Mechanism of Cancer Cell Death by Effective Anticancer Therapy

By the 1990s, apoptosis (44) , a physiological mechanism for controlled cell deletion that is an energy-dependent, inherent gene-directed program of cell death, sometimes referred to as cell suicide and programmed cell death, was considered the cause of anticancer agent-induced cancer cell death (45 , 46) . Apoptosis and necrosis are considered separate entities, not only morphologically but mechanistically. It is generally believed that clinically effective anticancer agents, despite having different primary biochemical targets, e.g., DNA damage by topoisomerase inhibitors, microtubule damage by paclitaxel and Taxotere, Fas antibody ligand binding to a Fas cell membrane surface receptor, and radiation damage to cell membrane sphingomyelin, all ultimately kill by inducing the biochemical cascades of apoptosis and necrosis (45 , 46) .

The sequential biochemical steps of apoptosis are schematically outlined in Fig. 2Citation . Mitochondria play a central role in apoptosis (47) . Anticancer agent-induced DNA damage effects a fall in the MPT (47 , 48) . The MPT fall releases apoptosis-inducing stimuli, reactive oxygen species, Bax (a proapoptotic protein), and Ca2+ overload (47 , 48) , are all factors that facilitate rupture of mitochondria. Mitochondrial rupture releases cytochrome c and procaspase-9 to join with cytosolic Apaf-1 and ATP in an apoptosome, leading to the activation of caspase-9 (49 , 50) . Activated caspase-9 then leads to other caspase-caspase interactions that activate caspase-3, caspase-6, and caspase-7 and the consequent cleavage of key substrates by the activated caspases (51 , 52) . Caspases, cysteine aspartate proteases, are active in proteolysis, and the result is the dismantling of the cell with the morphology of apoptosis (51 , 52) . Radiation injury to cell membrane sphingomyelin activates the sphingomyelin signaling system to induce apoptosis (53) . Ceramide is the second messenger of this pathway and is generated by hydrolysis of plasma membrane sphingomyelin through the action of either a neutral acidic sphingomyelinase (53) or by de novo synthesis via the enzyme ceramide synthase (54) . Bcl-2 and Bcl-xL are antiapoptotic proteins that protect mitochondria from loss of mitochondrial membrane potential (55 , 56) . The release of caspase-8 (48) by Fas activation leads to direct activation of the caspase system to cleave key substrates, dismantling the cell by apoptosis (51) . Caspase-8 can also activate the proapoptotic protein, Bid, that can lead to mitochondrial rupture with activation of the mitochondrial-induced caspase/apoptotic death response system (48 , 57) . Caspase-3 cleaves PARP, halting the pathway to ATP depletion-induced necrosis via PARP-induced NAD+ depletion (58 , 59) . Thus, the destruction of PARP activity permits caspase activity to complete apoptosis before PARP-induced ATP depletion causes necrotic cell death. It also should be noted that microtubule drugs induce apoptosis, and that there is evidence that interactions between the mitochondria and the cytoskeleton permit microtubule-active drugs to suppress the closure of the permeability transition pore in tumor mitochondria (60) .



View larger version (22K):
[in this window]
[in a new window]
[Download PPT slide]
  		Fig. 2. Schematic outline of sequential biochemical pathways to apoptosis induced by anticancer agents. Fas, cell surface membrane receptor; TNFR-1, tumor necrosis factor receptor-1; ROS, reactive oxygen species; Cyto c, cytochrome c; Mito, mitochondrial.

 
Controversy over ATP Depletion and Apoptosis

It is 28 years since Kerr et al. (in 1972; Ref. 44 ) first outlined the morphological criteria that distinguished cell death by apoptosis from necrosis. Many years passed before apoptosis became a biological subject of widespread and great scientific interest. Elucidation of its biochemical mechanism essentially began in the early 1990s. Thus, in the late 1980s, the preclinical therapeutic findings with the MAP program based on enhancing cell death by modulating ATP depletion was still compatible with the existing knowledge that necrosis was the mode of anticancer agent-induced cancer cell death.

However, by the early 1990s most clinically effective anticancer agents were considered to kill cancer cells by apoptosis (45 , 46) , and the presence of ATP was considered necessary for apoptosis (22 , 61, 62, 63) . For example, ATP is necessary for conversion of procaspase-9 to activated caspase-9 (50) . Thus, the remarkable antitumor effects of MAP attributed to MAP-induced ATP depletion was questioned.

New Facts and New Insights into the ATP-Depletion/Necrosis/Apoptosis Paradox

Although clinically effective anticancer agents frequently kill cancer cells by activation of the biochemical cascade of apoptosis (45 , 46) , the same anticancer agents can induce cancer cell death by necrosis (56 , 64 , 65) . Moreover, these two modes of cell death can occur in different cells simultaneously in tumors and cell cultures exposed to the same agent (56 , 64 , 65) . The particular mode of cell death induced after drug treatment is dependent on the drug, its concentration, and the particular cell line (65) . Because ATP depletion is the cause of necrosis, whereas ATP is necessary for apoptosis, it is noteworthy that necrotic and apoptotic cell death occur in the same tumor (but in different cells) after anticancer treatment. One reason is that different drug concentrations reach different cancer cells; low concentrations induce apoptosis, and higher concentrations cause necrotic cell death (65) . However, this is not the only reason.

Because activated caspases execute apoptosis, it is noteworthy that the apoptotic mode of cell death can be prevented by an inhibitor of caspases (e.g., Z-VAD-fmk), but instead of cell survival there is a shift to the necrotic mode of cell death (66, 67, 68, 69, 70, 71, 72) . The reason is that severe ATP depletion, causative of necrosis, is brought about both by the fall in MPT (52) , effecting a cessation of mitochondrial oxidative phosphorylation that generates ATP, as well as the block of caspase-3 by Z-VAD-fmk preventing caspase-3 cleavage of PARP, the result being continued PARP activity leading to NAD+ depletion and consequent ATP depletion.

It is important to note that there are genetic deletions of caspases (73 , 74) , and there are endogenous IAP, i.e., caspase inhibitors (75) . Because apoptosis is governed by activated caspases, genetic loss of caspases or block by IAP of caspase activity, prevents apoptosis. In Fig. 3Citation , caspase inhibition by IAPs plus continued activity by PARP (note in Fig. 3Citation , PARP cleavage by caspase-3 is blocked by an IAP), plus the ATP depletion from the loss of electron transport in ruptured mitochondria, drive the cell to necrosis largely because of continuation of PARP-induced ATP depletion (52 , 76) . It is believed that the purpose of PARP cleavage is to prevent induction of necrosis during apoptosis and ensure appropriate execution of caspase-mediated apoptosis (76) . Failure of PARP cleavage (e.g., by IAP-blocked caspases) would be expected to lead to the increased induction of necrosis but, surprisingly, is also reported to enhance apoptosis (58 , 76) . The question marks in Fig. 3Citation indicate that whether this enhancement is influenced by the continued PARP synthesis of PAR or by a relationship to the NAD+ level is not understood (58 , 76) .



View larger version (29K):
[in this window]
[in a new window]
[Download PPT slide]
  		Fig. 3. Schematic outline of necrotic and apoptotic pathways with endogenous inhibitors of apoptosis, IAP, i.e., inhibitors of caspases (75) . If PARP cleavage is prevented, the continued activity of PARP leads to enhancement of both necrosis and apoptosis (58 , 76) . ?, the possible relevance of NAD+ levels and PAR, poly(ADP-ribose) polymers, to the enhanced apoptosis is not known.

 
In brief, intracellular ATP levels may determine whether anticancer agent-induced cell death fate is by necrosis or apoptosis (77 , 78) . The activation and action of caspases, before ATP depletion can fall to levels causing cell death by necrosis, allows for caspase-executed apoptosis, and the availability of caspases versus IAP can dictate the propensity of cells to die from apoptosis versus necrosis. There are many reports of inhibition of caspase activity not conferring a survival advantage because the result is a shift from apoptotic cell death to necrotic cell death (22 , 52 , 56 , 63 , 64 , 66, 67, 68, 69, 70, 71, 72 , 77 , 78) .

A recent review article on mitochondria and apoptosis (52) states that, "The emergent view is that once cytochrome c is released ... (by mitochondrial rupture) ... , this commits the cells to die by either an apoptotic mechanism involving Apaf-1-mediated caspase activation or a slower necrotic process due to collapse of electron transport, which occurs when Cyto C is depleted from mitochondria resulting in a variety of deleterious sequelae including generation of oxygen free radicals and decreased production of ATP."

All of the above observations reveal that, rather than functional opposition between the two types of cell death, necrosis and apoptosis, there is a functional cooperativity (Fig. 3)Citation . The therapeutic implications are that a heterogeneous neoplastic cell population of a tumor likely includes cells with IAP, gene deletions of certain caspases, and lower levels of Bax. These cancer cells are likely to be of lesser sensitivity to an anticancer agent and escape death because they do not receive enough damage to reduce ATP to levels low enough to be insufficient to support cell viability. The insight provided by the findings noted above and in Fig. 3Citation suggests that biochemical modulation to further depress ATP to still lower levels than that induced by the anticancer agent alone would kill these sublethally injured cells, augment tumor regressions, and even yield some cures. The preclinical enhanced therapeutic results with MAP + anticancer agents support this thesis.

One new understanding of the paradox in obtaining improved therapeutic results by adding ATP-depleting modulatory treatment to the ATP-requiring apoptotic process is that necrosis and apoptosis are sometimes not completely separate entities in a cancer cell "hit" by an anticancer agent. Both modes of cell death are simultaneously induced by the DNA damage; more specifically, PARP activation as well as mitochondrial damage by a fall in the MPT (Fig. 3)Citation . If PARP cleavage occurs by activated caspase-3, necrosis is prevented and apoptosis prevails. If PARP cleavage is prevented by an IAP, necrosis prevails with an assist in ATP depletion from the apoptotically damaged mitochondria in the ongoing process of necrosis. It is understandable that ATP-depleting modulatory therapy would enhance necrosis and improve the therapeutic results. However, under conditions where PARP activity continues (i.e., PAR synthesis and NAD+ consumption continues), not only is there increased necrosis, but surprisingly, apoptosis also increases (58 , 76) . The latter situation (i.e., uncleaved PARP leading to increased apoptosis) is not understood. Perhaps the continued activity of PARP induces changes in the pyridine nucleotide pool (NADH/NAD + NADPH/NADP) and nucleotide pool of ADP and ATP that regulate MPT (71 , 79) , leading to a fall in the MPT of additional mitochondria that affects rupture of these mitochondria-releasing apoptogenic factors that result in increased caspase activity and increased apoptosis. Further research will hopefully explain the question mark in Fig. 3Citation . If these conjectures apply, the MAP regimen (i.e., its NAD+ antagonist and ATP) could similarly influence the MPT and increase apoptosis.

ATP Depletion Is the Primary Mechanism of MAP.

Most pertinent to the question of whether the MMPR + 6-AN mechanism of enhancing ATP depletion has anything to do with enhancing tumor regressions is the demonstration that MMPR alone can reduce ATP levels to 34% in murine breast tumors, but in combination with 6-AN the ATP level is further reduced to 15% of normal (28) . Importantly, this low level of ATP, 15%, cannot sustain cell viability (20 , 21) , and tumor regressions ensue. Also of relevance to ATP depletion and cell death, the combination of MMPR + 6-AN has been demonstrated to initiate a significant depletion of ATP prior to the onset of cell death (27) .

There is published data (80) comparing both the therapeutic results and the ATP-depleting effect of MAP alone, MAP + FU, MAP + Adr, and MAP + FU + Adr. ATP depletion becomes more profound in conjunction with increasing levels of tumor-regressing therapeutic activity as treatment is increased from MAP, to MAP + FU or MAP + Adr, to MAP + FU + Adr; the latter levels of ATP depletion and tumor regression rates were significantly lower than that observed in tumors from mice treated with MAP + FU or MAP + Adr (80) . Thus, a positive correlation was found between increasing levels of ATP depletion and increasing tumor regression. In other studies (81) , both the depletion of ATP by MAP + Adr and tumor regressions were significantly greater than that of MAP alone. Thus, this correlative quantitative data supports ATP depletion as a significant factor in the production of tumor regressions.

The recent reports that blocking activated caspases by exogenous caspase inhibitors (Z-VAD-fmk; Refs. 22 , 56 , 64 , 66, 67, 68, 69, 70, 71, 72 , 77 , 78 ) or endogenous inhibitors (IAPs; Ref. 52 ) prevents the apoptotic mode of cell death but causes the ATP-depleting form of cell death, necrosis, clearly demonstrate that ATP depletion can be made into a primary effector of cell death. Manipulation of cellular energy metabolism (e.g., inhibition of the mitochondrial respiratory chain or provision or withdrawal of substrates for glycolysis) shifts the balance between apoptosis and necrosis (22) . All of these shifts to death by necrosis are physiological effects attributable to severe ATP depletion; very low levels of ATP cannot sustain cell viability (20 , 21) .

Taken together, all of the above facts are compelling evidence that the enhanced antitumor effects observed in our studies are the result of ATP depletion. Similar therapeutic gains have been obtained by concomitantly administering MAP with nine different DNA-damaging agents that, although they damage DNA by different mechanisms, induce in common the same processes of apoptosis and necrosis that evoke ATP depletion. Hence, cancer cells sublethally injured because of the DNA-damaging agents will have various degrees of ATP depletion that can be further reduced by MAP to cell-killing levels. It seems clear that ATP depletion is the critical biochemical event common to the cell deaths induced by nine mechanistically different anticancer agents when given with MAP.

Mechanisms of action other than ATP depletion have been ascribed to MMPR and 6-AN. MMPR, as a single agent, is reported to act as an inhibitor of tumor vascularization but did not kill cancer cells or cause tumor regression (82) . 6-AN, as a single agent, is reported to up-regulate the glucose-regulated stress protein, GRP 78, a finding associated with potentiation of cytotoxicity in vitro of certain anticancer agents; however, the effect of 6-AN on ATP depletion, which is the likely cause of the enhanced cytotoxicity, was not measured (83) . Multiple mechanisms of action have been demonstrated for almost all anticancer agents. For example, doxorubicin has had at least nine mechanisms demonstrated, but the interaction with topoisomerase II is nevertheless considered the primary triggering event for cell killing through apoptosis (84) . The primary mechanism of action for the enhanced antitumor effect obtained by MAP plus an anticancer agent is clearly severe ATP depletion.

Proposed Clinical Trial of MAP

A proposed clinical trial of MAP has potential for a treatment advance in cancer patient care. Single agent 6-AN has been administered in three Phase I clinical trials in patients with disseminated cancer (85, 86, 87) , and these studies demonstrated that 6-AN toxicity takes two clinical forms, a low-dose, mixed B complex vitamin deficiency and a high-dose-dependent central nervous system toxicity. Of note in the early clinical studies, 6-AN was given daily, whereas the proposed clinical trial for MAP is an infrequent intermittent schedule every 2 weeks; this toxicity should be much less.

It is the preclinically proven, ATP-depleting modulatory concept that requires appropriate clinical exploration and not specific drugs. Thus, the clinical trial need not necessarily be done with the MAP regimen to prove the therapeutic value of the ATP depletion concept at the clinical level. However, the MAP regimen seems a reasonable first choice, not only for the basic scientific data and reasons already given, and the successful preclinical data with MAP, but because a MAP clinical trial could be completed in a relatively short time. All three of the MAP drugs have been independently evaluated clinically, and therefore, their toxicities and some schedules are known. Cancer patients have received MMPR + PALA combined in a single regimen with a concomitantly administered anticancer drug, FU (88) . Thus, evaluating the MAP regimen in the clinic merely requires integration of 6-AN into the clinically established MMPR + PALA regimen. Clearly, less time would be required for evaluating MAP in the clinic compared with new agents.

Conclusions

(a) Preclinical in vivo tumor studies have demonstrated that a combination of ATP-depleting agents (that reduce tumor cell ATP levels to <15% of normal) administered with anticancer agent therapy markedly enhanced tumor regressions and can even produce cures.

(b) Because of the knowledge of the basic mechanisms effecting necrosis and apoptosis and their interrelationships, the correlation of MAP-induced ATP depletion with MAP-induced tumor regressions, and the marked enhancement of preclinical anticancer activity by the concomitant administration of MAP + nine mechanistically different anticancer agents, the total data merit a MAP trial at the clinical level.

(c) At the preclinical level, the therapeutic opportunity opened by modulation of NAD+ and ATP levels merits further research. Other pharmacological manipulations may further improve the MAP regimen.

ACKNOWLEDGMENTS

We give grateful acknowledgment to Dr. Larry Norton, Memorial Sloan-Kettering Cancer Center, for his interest, support, and encouragement of this work.

FOOTNOTES

The costs of publication of this article were defrayed in part by the payment of page charges. This article must therefore be hereby marked advertisement in accordance with 18 U.S.C. Section 1734 solely to indicate this fact.

1 Supported by the Breast Cancer Research Foundation, and NIH R24 Ca 83084-01. Back

2 To whom requests for reprints should be addressed, at Memorial Sloan-Kettering Cancer Center, Box 84, 1275 York Ave, New York, NY 10021. Phone: (212) 639-8835; Fax: (212) 717-3676. Back

3 The abbreviations used are: PARP, poly(ADP-ribose) polymerase; 6-AN, 6-aminonicotinamide; MMPR, 6-methylmercaptopurine riboside; MMPR-P, MMPR-phosphate; PALA, N-(phosphonacetyl)-L-aspartic acid; PR, partial regression; MAP, MMPR + 6-AN + PALA; FU, 5-fluorouracil; Adr, Adriamycin; MTAP, methylthioadenosine phosphorylase; MPT, mitochondrial permeability transition; IAPS, inhibitor(s) of apoptosis. Back

4 Unpublished results. Back

Received 2/25/00. Accepted 10/18/00.

REFERENCES

  1. Martin D. S. Biochemical modulation: perspectives and objectives Harrap K. R. eds. . New Avenues in Developmental Cancer Chemotherapy, : 113-162, Academic Press London 1986.
  2. Berger N. A., Berger S. J. Metabolic consequences of DNA damage: the role of poly (ADP-ribose) polymerase as mediator of the suicide response Grossman L. Upton A. C. eds. . Mechanisms of DNA Damage and Repair, : 357-363, Plenum Publishing Corp. New York 1986.
  3. Tanizawa A., Kubota M., Hashimoto H., Shimizu T., Takimoto T., Kitoh T., Akiyama Y., Mikama H. VP-16-induced nucleotide pool changes and poly (ADP-ribose) synthesis: the role of VP-16 in interphase death. Exp. Cell Res., 185: 237-246, 1989.[Medline]
  4. Carson D. A., Seto S., Wasson B., Carrera C. DNA strand breaks, NAD metabolism, programmed cell death. Exp. Cell. Res., 164: 273-281, 1986.[Medline]
  5. Schraufstaffer I. U., Hinshaw D. B., Hyslop P. S., Spragg R. H., Cochrane C. G. Oxidant injury of cells DNA stand-breaks activate polyadenosine diphosphate polymerase and lead to depletion of nicotinamide adenine dinucleotide. J. Clin. Investig., 77: 1312-1320, 1986.
  6. Gaal J. C., Smith K. R., Pearson C. K. Cellular euthanasia mediated by a nuclear enzyme: a central role for nuclear ADP-ribosylation in cellular metabolism. Trends Biochem. Sci., 12: 129-132, 1987.
  7. Marks D. I., Fox R. M. DNA damage, poly(ADP-ribosyl)ation and apoptotic cell death as a potential common pathway of cytotoxic drug action. Biochem. Pharmacol., 42: 1859-1867, 1991.[Medline]
  8. Dietrich L. S., Kaplan L., Friedland I. M. Pyridine nucleotide metabolism: mechanism of action of the niacin antagonist, 6-aminonicotinamide. J. Biol. Chem., 233: 964-968, 1958.[Free Full Text]
  9. Varnes M. E. Inhibition of pentose cycle of A54 cells by 6-aminonicotinamide: consequences for aerobic and hypoxic radiation response and for radiosensitizer action. Natl. Cancer Inst. Monogr., 6: 199-202, 1988.
  10. Herken H., Lange K., Kolbe H. Brain disorder induced by pharmacological blockade of the pentose phosphate pathway. Biochem. Biophys. Res. Commun., 36: 93-100, 1969.[Medline]
  11. Hunting D., Gowans B., Henderson J. F. Effects of 6-AN on cell growth, poly(ADP-ribose) synthesis and nucleotide metabolism. Biochem. Pharmacol., 34: 3999-4003, 1985.[Medline]
  12. Street J. C., Mahmoud V., Ballon D., Alfieri A. A., Koutcher J. A. 13C and 31P NMR investigation of effect of 6-aminonicotinamide on metabolism of RIF-1 tumor cells in vitro. J. Biol. Chem., 271: 4113-4119, 1996.[Abstract/Free Full Text]
  13. Koutcher J. A., Alfieri A. A., Matei C., Zakian K. L., Street J. C., Martin D. S. In vivo 31P NMR detection of pentose phosphate pathway block and enhancement of radiation sensitivity with 6-aminonicotinamide. Magn. Reson. Med., 36: 887-892, 1996.[Medline]
  14. Shantz G. D., Smith C. M., Fontenella L. J., Lau H. K. F., Henderson J. F. Inhibition of purine nucleotide metabolism by 6-methylmercaptopurine ribonucleoside and structurally related compounds. Cancer Res., 33: 2867-2871, 1973.[Abstract/Free Full Text]
  15. Warnick C. T., Patterson A. R. P. Effect of methylthioinosine on nucleoside concentration in L5158 cells. Cancer Res., 33: 1711-1715, 1973.[Abstract/Free Full Text]
  16. Grindey G. B., Lowe J. K., Divekey A. Y., Hakala M. T. Potentiation by guanine nucleosides of the growth-inhibitory effects of adenosine analogues on L1210 and Sarcoma 180 cells in culture. Cancer Res., 36: 379-383, 1976.[Abstract/Free Full Text]
  17. Martin D. S., Stofli R. L., Sawyer R. C., Spiegelman S., Casper E. S., Young C. W. Therapeutic utility of utilizing low doses of N-(phosphonacetyl)-L-aspartic acid in combination with 5-fluorouracil: a murine study with clinical relevance. Cancer Res., 43: 2317-2321, 1983.[Abstract/Free Full Text]
  18. Martin D. S. Purine and pyrimidine biochemistry, and some relevant clinical and preclinical cancer chemotherapy research Powis G. Prough R. A. eds. . Metabolism and Action of Anti-Cancer Drugs, : 91-140, Talyor & Francis London 1987.
  19. Martin D. S. Cancer chemotherapy: past is prologue. Mt. Sinai. J. Med., 52: 426-434, 1985.[Medline]
  20. Nieminen A. L., Saylor A., Herman B., Lemasters J. J. ATP depletion rather than mitochondrial depolarization mediates hepatocyte killing after metabolic inhibition. Am. J. Physiol, 267: C67-C74, 1994.[Abstract/Free Full Text]
  21. Sweet S., Singh G. Accumulation of human promyelocytic leukemic (HL-60) cells at two energetic cell cycle checkpoints. Cancer Res., 55: 5164-5167, 1995.[Abstract/Free Full Text]
  22. Nicotera P., Leist M. Energy supply and the shape of death in neurons and lymphoid cells. Cell Death Differ., 4: 435-442, 1997.
  23. Stolfi R. L., Martin D. S., Fugman R. A. Spontaneous murine mammary adenocarcinoma: model system for the evaluation of combined methods of therapy. Cancer Chemother. Rep. Part 1, 55: 239 1971.[Medline]
  24. Martin D. S., Fugman R. A., Stolfi R. L., Hayworth E. Solid tumor animal model therapeutically predictive for human breast cancer. Cancer Chemother. Rep. Part 2, 5: 89 1975.
  25. Goldin A., Kendetti J. M., MacDonald J. S., Muggia F., Henney J., DeVita V. T. Current results of the screening program at the Division of Cancer Treatment, National Cancer Institute. Eur. J. Cancer, 17: 129 1981.
  26. King M. P., Attardi G. Human cells lacking mtDNA: repopulation with exogenous mitochondria by complementation. Science (Washington DC), 246: 500-503, 1989.[Abstract/Free Full Text]
  27. Nord L. D., Stolfi R. L., Alfieri A. A., Netto G., Reuter V., Sternberg S. S., Colofiore J. R., Koutcher J. A., Martin D. S. Apoptosis induced in advanced CD8F1-murine mammary tumors by the combination of PALA, MMPR and 6-AN precedes tumor regression and is preceded by ATP depletion. Cancer Chemother. Pharmacol., 40: 376-384, 1997.[Medline]
  28. Martin D. S., Stolfi R. L., Colofiore J. R. Perspective. The chemotherapeutic relevance of apoptosis and a proposed biochemical cascade for chemotherapeutically induced apoptosis. Cancer Investig., 15: 372-381, 1997.[Medline]
  29. Koutcher J. A., Alfieri A., Stolfi R. L., Devitt M. L., Colofiore J. R., Nord L. D., Martin D. S. Potentiation of a three drug chemotherapy regimen by radiation. Cancer Res., 53: 3518-3823, 1993.[Abstract/Free Full Text]
  30. Stolfi R. L., Colofiore J. R., Nord L. D., Koutcher J. A., Martin D. S. Biochemical modulation of tumor cell energy: regression of advanced spontaneous murine breast tumors with a 5-fluorouracil containing drug combination. Cancer Res., 52: 4074-4981, 1992.[Abstract/Free Full Text]
  31. Martin D. S., Stolfi R. L., Colofiore J. R., Nord L. D., Sternberg S. Biochemical modulation of tumor cell energy in vivo. II. A lower dose of Adriamycin is required and a greater antitumor activity is induced when cellular energy is depressed. Cancer Investig., 12: 296-307, 1994.[Medline]
  32. Stolfi R. L., Colofiore J. R., Nord L. D., Martin D. S. Enhanced antitumor activity of an Adriamycin + 5-fluorouracil combination when preceded by biochemical modulation. Anti-Cancer Drugs, 7: 100-104, 1996.[Medline]
  33. Martin, D. S., Stolfi, R. L., Colofiore, J. C., Koutcher, J. A., Alfieri, A., Sternberg, S., and Nord, L. D. Apoptosis resulting from anti-cancer agent activity in vivo is enhanced by biochemical modulation of tumor cell energy. In: M. Lavin and D. Walters (eds.), Programmed Cell Death. The Cellular and Molecular Biology of Apoptosis, pp. 279–296. New York: Harwood Academic, 1993.
  34. Martin, D. S., Spriggs, D., and Koutcher, J. A. Aminonicotinamide (6-AN), alone, or in combination with 6-methylmercaptopurine riboside (MMPR) and PALA, markedly enhances cisplatin-induced anticancer activity. Apoptosis, in press, 2001.
  35. Martin D. S., Stolfi R. L., Nord L. D., Colofiore J. R. Enhancement of chemotherapeutically-induced apoptosis in vivo by biochemical modulation of poly(ADP-ribose) polymerase. Oncol. Rep., 3: 317-322, 1996.
  36. Martin D. S., Stolfi R. L., Colofiore J. R., Nord L. D. Marked enhancement in vivo of paclitaxel’s (Taxol’s) tumor-regressing activity by ATP-depleting modulation. Anti-Cancer Drugs, 7: 655-659, 1996.[Medline]
  37. Kamatani N., Nelson-Rees W. A., Carson D. A. Selective killing of human malignant cell lines deficient in methylthioadenosine phosphorylase, a purine metabolic enzyme. Proc. Natl. Acad. Sci. USA, 78: 1219-1223, 1981.[Abstract/Free Full Text]
  38. Fitchen J. H., Riscoe M. K., Dana B. W., Lawrence H. J., Ferro A. J. Methylthioadenosine phosphorylase deficiency in human leukemias and solid tumors. Cancer Res., 46: 5409-5412, 1986.[Abstract/Free Full Text]
  39. Nobori T., Karras J. G., Della Ragione F., Waltz T. Z., Chen P. P., Carson D. A. Absence of methylthioadenosine phosphorylase in human gliomas. Cancer Res., 51: 3193-3197, 1991.[Abstract/Free Full Text]
  40. Nobori T., Szinai I., Amox D., Parker B., Olopade O. I., Buchhagen D. L., Carson D. A. Methylthioadenosine phosphorylase deficiency in human non-small cell lung cancers. Cancer Res., 53: 1098-1101, 1993.[Abstract/Free Full Text]
  41. Chen Z. H., Zhang H., Savarese T. M. Gene deletion chemoselectivity: codeletion of the genes for p16INK4, methylthioadenosine phosphorylase, and the {alpha}- and ß-interferons in human pancreatic cell carcinoma lines and its implications for chemotherapy. Cancer Res., 56: 1083-1090, 1996.[Abstract/Free Full Text]
  42. Batova A., Diccianni M. B., Omura, Minamisawa M., Yu J., Carrera C. J., Bridgeman L. J., Kung F. H., Pullen J., Amyulon M. D., Yu A. L. Use of alanosine as a methyladenosine phosphorylase–selective therapy for T-cell acute lymphoblastic leukemia in vitro. Cancer Res., 59: 1492-1497, 1999.[Abstract/Free Full Text]
  43. Li W. W., Cole P., Martin D., Banerjee D., Bertino J. R. Methylthioadenosine phosphorylase (MTAP) status determines sensitivity to L-alanosine in human soft tissue sarcoma cell lines and is enhanced by 6-methylmercaptopurine riboside (MMPR). Proc. Am. Assoc. Cancer Res., 41: 240 2000.
  44. Kerr J. F. R., Wyllie A. H., Currie A. R. Apoptosis: a basic biological phenomenon with wide-ranging implications in tissue kinetics. Br. J. Cancer, 26: 239-257, 1972.[Medline]
  45. Hickman J. A. Apoptosis induced by anticancer drugs. Cancer Metastasis Rev., 11: 121-139, 1992.[Medline]
  46. Reed J. C. Regulation of apoptosis by bcl-2 family proteins and its role in cancer and drug resistance. Curr. Opin. Oncol., 7: 541-546, 1995.[Medline]
  47. Kroemer G., Zamzami N., Susin S. A. Mitochondrial control of apoptosis. Immunol. Today, 18: 44-51, 1997.[Medline]
  48. Green D. R. Apoptotic pathways: the roads to ruin. Cell, 94: 695-698, 1998.[Medline]
  49. Zou H., Li Y., Liu X., Wang X. An apaf-1-cytochrome c multimeric complex is a functional apoptosome that activates procaspase-9. J. Biol. Chem., 274: 11549-11556, 1999.[Abstract/Free Full Text]
  50. Liu X., Kim C. N., Yang J., Jemmerson R., Wang X. Induction of apoptotic program in cell-free extracts: requirement for dATP and cytochrome c. Cell, 86: 147-157, 1996.[Medline]
  51. Schmitt E., Sane A. T., Bertrand R. Activation and role of caspases in chemotherapy-induced apoptosis. Drug Resistance Updates, 2: 21-29, 1999.[Medline]
  52. Green D. R., Reed J. C. Mitochondria and apoptosis. Science (Washington DC), 281: 1309-1312, 1998.[Abstract/Free Full Text]
  53. Haimovitz-Friedman A., Kan C. C., Ehleiter D., Persaud R. S., McLoughlin M., Fuks Z., Kolesnick R. N. Ionizing radiation acts on cellular membranes to generate ceramide and initiate apoptosis. J. Exp. Med., 180: 525-535, 1994.[Abstract/Free Full Text]
  54. Bose R., Verheij M., Haimovitz-Friedman A., Scotto K., Fuks Z., Kolesnick R. Ceramide synthase mediates daunorubicin-induced apoptosis: an alternative mechanism for generating death signals. Cell, 82: 405-411, 1995.[Medline]
  55. Susin S. A., Zamzami N., Castedo M., Hirsch T., Marchetti P., Macho A., Dauges E., Gauskens M., Kroemer G. Bcl-2 inhibits the mitochondrial release of an apoptogenic protease. J. Exp. Med., 184: 1331-1342, 1996.[Abstract/Free Full Text]
  56. Shimizu S., Equchi V., Kamike W., Itoh Y., Hasegawa J., Yamabe K., Otsuid Y., Matsuda H., Tsujimoto Y. Induction of apoptosis as well as necrosis by hypoxia and predominant prevention of apoptosis by bcl-2 and bcl-x. Cancer Res., 56: 2161-2166, 1997.[Abstract/Free Full Text]
  57. Li H., Zhu H., Xu C. J. Cleavage of BID by caspase 8 mediates the mitochondrial damage in the Fas pathway of apoptosis. Cell, 94: 491-501, 1998.[Medline]
  58. Boulares A. H., Yokovlev A. G., Ivanova V., Stoica B. A., Wang G., Iyer S., Smulson M. Role of poly(ADP-ribose) polymerase (PARP) cleavage in apoptosis. Caspase-3 resistant PARP mutant increases rates of apoptosis in transfected cells. J. Biol. Chem., 274: 22932-22940, 1999.[Abstract/Free Full Text]
  59. Janicke R. V., Sprengart M. L., Wati M. R., Porter A. G. Caspase-3 is required for DNA fragmentation and morphological changes associated with apoptosis. J. Biol. Chem., 273: 9357-9360, 1998.[Abstract/Free Full Text]
  60. Evtodienko Y. V., Teplova V. V., Sidosh S. S., Ichas F., Mazal J. P. Microtubule-active drugs suppress the closure of the permeability transition pore in tumor mitochondria. FEBS Lett., 393: 86-88, 1996.[Medline]
  61. Cotter T. G., Lenon S. V., Glynn J. G., Martin S. J. Cell death via apoptosis and its relationship to growth, development and differentiation of both tumor and normal cells. Anticancer Res., 10: 1153-1160, 1990.[Medline]
  62. Wyllie A. H. Apoptosis. Br. J. Cancer, 67: 205-208, 1993.[Medline]
  63. Nicotera P., Leist M. Mitochondrial signals and energy requirement in cell death. Cell Death Differ., 4: 516 1997.
  64. Amarante-Mendes G. P., Finucane D. M., Martin S. J., Cotter T. G., Salvesen G. S., Green D. R. Anti-apoptotic oncogenes prevent caspase-dependent and independent commitment for cell death. Cell Death Differ., 5: 298-306, 1998.[Medline]
  65. Huschtscha L. I., Andersson C. E., Bartier W. A., Tattersall M. H. N. Anti-cancer drugs and apoptosis Lavin M. Walters D. eds. . Programmed Cell Death, the Cellular and Molecular Biology of Apoptosis, : 269-278, Harwood Academic New York 1993.
  66. Sane A. T., Bertrand R. Caspase inhibition in camptothecin-treated U-937 cells is completed with a shift from apoptosis to transient G, arrest followed by necrotic cell death. Cancer Res., 59: 3565-3569, 1999.[Abstract/Free Full Text]
  67. Lemaire C., Andreau K., Souvannavong K., Adam A. Inhibition of caspase activity induces a switch from apoptosis to necrosis. FEBS Lett., 425: 266-270, 1998.[Medline]
  68. Cappola S., Nosseri C., Maresco V., Ghibelli L. Different basal NAD levels determine opposite effects of poly(ADP-ribosyl) polymerase inhibitors on H2O2-induced apoptosis. Exp. Cell Res., 221: 462-469, 1995.[Medline]
  69. Kiang J., Chao T., Korsmyer S. J. Bax-induced cell death may not require interleukin 1-converting enzyme-like proteases. Proc. Natl. Acad. Sci. USA, 93: 143559-14563, 1996.
  70. Shimizu S., Equchi Y., Kamuke W., Waguri S., Vchiyama Y., Matsuda H., Tsujimoto Y. Bcl-2 blocks loss of mitochondrial membrane potential with ICE inhibitors act at a different step during inhibition of death induced by respiratory chain inhibitors. Oncogene, 13: 21-29, 1996.[Medline]
  71. Hirsch T., Marchetti P., Susin S., Dellaporta B., Zamzami N., Marzo I., Geuskens M., Kroemer G. The apoptosis-necrosis paradox. Apoptogenic proteases activated after mitochondrial permeability transition determine the mode of cell death. Oncogene, 15: 1573-1581, 1997.[Medline]
  72. Mehmet H., Yue X., Penrice J., Cady E., Wyatt J. S., Surraf C., Squier M., Edwards A. D. Relation of impaired energy metabolism to apoptosis and necrosis following transient cerebral hypoxia-ischemia. Cell Death Differ., 5: 321-329, 1998.[Medline]
  73. Kuida K., Hayder T. F., Kuan C. Y., Gu Y., Taya C., Karasuyama H., Su M. S. S., Radic P., Flavell R. A. Reduced apoptosis and cytochrome c-mediated caspase activation in mice lacking caspase activation in mice lacking caspase 9. Cell, 94: 325-337, 1998.[Medline]
  74. Yoshida H., Kong Y. Y., Yoshida R., Elia A. J., Hakem R., Penninger J. M., Mak T. W. Apaf-1 is required for mitochondrial pathways of apoptosis and brain development. Cell, 94: 739-750, 1998.[Medline]
  75. Roy N., Dveraux Q. L., Takahashi R., Salvesen G. S., Reed J. C. The c-IAP-1 and c-IAP-2 proteins are direct inhibitors of specific caspases. EMBO J., 16: 6914-6925, 1997.[Medline]
  76. Herceg Z., Wang Z. Q. Failure of poly(ADP-ribose) polymerase cleavage by caspases leads to induction of necrosis and enhanced apoptosis. Mol. Cell Biol., 19: 5124-5133, 1999.[Abstract/Free Full Text]
  77. Eguchi Y., Shimizu S., Tsujimoto Y. Intracellular ATP levels determine cell fate by apoptosis or necrosis. Cancer Res., 57: 1835-1840, 1997.[Abstract/Free Full Text]
  78. Leist M., Single B., Castoldi A. F., Kuknle S., Nicotera P. Intracellular triphosphate (ATP) concentration: a switch in the decision between apoptosis and necrosis. J. Exp. Med., 185: 1481-1486, 1997.[Abstract/Free Full Text]
  79. Constantini P., Chernyak B. V., Petronilli V., Bernardi P. Modulation of the mitochondrial permeability transition pore by pyridine nucleotides and dithiol oxidation at two separate sites. J. Biol. Chem., 271: 6746-6751, 1996.[Abstract/Free Full Text]
  80. Colofiore J. R., Stolfi R. L., Nord L. D., Martin D. S. On the relationship of ATP depletion to chemotherapeutically-induced tumor regression. Int. J. Oncol., 7: 1401-1404, 1995.
  81. Colofiore J. R., Stolfi R. L., Nord L. D., Martin D. S. Biochemical modulation of tumor cell energy IV. Evidence for the contribution of adenosine triphosphate (ATP) depletion to chemotherapeutically-induced tumor regression. Biochem. Pharmacol., 50: 1943-1948, 1995.[Medline]
  82. Presto M., Rusunati M., Belleri M., Morbedelli L., Ziche M., Ribatti D. Purine analog 6-methylmercaptopurine riboside inhibits early and late phases of the angiogenesis process. Cancer Res., 59: 2417-2424, 1999.[Abstract/Free Full Text]
  83. Chatterjee S., Hirota H., Belfi C. A., Berger S. J., Berger N. A. Hypersensitivity to DNA cross-linking agents associated with up-regulation of glucose-regulated stress protein GRP 78. Cancer Res., 57: 5112-5116, 1997.[Abstract/Free Full Text]
  84. Gerwirtz D. A. A critical evaluation of mechanisms of action proposed for the antitumor effects of the anthracycline antibiotics Adriamycin and daunorubicin. Biochem. Pharmacol., 57: 727-741, 1999.[Medline]
  85. Taylor, S. G., Korman, S., Sky-Peck, H. H., and Perlia, C. 6-Aminonicotinamide in disseminated human cancer. Lab. Clin. Med., p. 950, 1958.
  86. Herter F., Weissman S. G., Thompson H. G., Hyman G., Martin D. S. Clinical experience with 6-aminonicotinamide. Cancer Res., 21: 31-37, 1961.
  87. Perlia C. P., Kofman S., Sky-Peck H., Taylor S. Clinical use of 6-aminonicotinamide in patients with disseminated neoplastic disease. Cancer, 14: 644-648, 1961.
  88. O’Dwyer P. J., Hudas G. R., Colofiore J., Walczak J., Hoffman J., La Creta F. P., Comis R. L., Martin D. S., Ozols R. F. Phase I trial of fluorouracil modulation by N-phosphonacetyl-L-aspartate and 6-methylmercaptopurine riboside: optimization of 6-methylmercaptopurine dose and schedule through biochemical analysis of sequential tumor biopsy specimens. J. Natl. Cancer Inst., 83: 1235-1240, 1991.[Abstract/Free Full Text]



This article has been cited by other articles:


Home page
 Hum Mol GenetHome page
G. P. Lobo, K. A. Waite, S. M. Planchon, T. Romigh, J. A. Houghton, and C. Eng
ATP modulates PTEN subcellular localization in multiple cancer cell lines
Hum. Mol. Genet., September 15, 2008; 17(18): 2877 - 2885.
[Abstract] [Full Text] [PDF]

Home page
 Clin. Cancer Res.Home page
S. Cao, F. A. Durrani, and Y. M. Rustum
Selective Modulation of the Therapeutic Efficacy of Anticancer Drugs by Selenium Containing Compounds against Human Tumor Xenografts
Clin. Cancer Res., April 1, 2004; 10(7): 2561 - 2569.
[Abstract] [Full Text] [PDF]

Home page
 Mol. Pharmacol.Home page
P. A. Nguewa, M. A. Fuertes, C. Alonso, and J. M. Perez
Pharmacological Modulation of Poly(ADP-ribose) Polymerase-Mediated Cell Death: Exploitation in Cancer Chemotherapy
Mol. Pharmacol., November 1, 2003; 64(5): 1007 - 1014.
[Full Text] [PDF]

Home page
 Mol Cancer ResHome page
N. V. Oleinik and S. A. Krupenko
Ectopic Expression of 10-Formyltetrahydrofolate Dehydrogenase in A549 Cells Induces G1 Cell Cycle Arrest and Apoptosis
Mol. Cancer Res., June 1, 2003; 1(8): 577 - 588.
[Abstract] [Full Text] [PDF]

Home page
 Cancer Res.Home page
J.-D. Jiang, L. Denner, Y.-H. Ling, J.-N. Li, A. Davis, Y. Wang, Y. Li, J. Roboz, L.-G. Wang, R. Perez-Soler, et al.
Double Blockade of Cell Cycle at G1-S Transition and M Phase by 3-Iodoacetamido Benzoyl Ethyl Ester, a New Type of Tubulin Ligand
Cancer Res., November 1, 2002; 62(21): 6080 - 6088.
[Abstract] [Full Text] [PDF]

Home page
 J. Biol. Chem.Home page
H. Mizutani, S. Tada-Oikawa, Y. Hiraku, S. Oikawa, M. Kojima, and S. Kawanishi
Mechanism of Apoptosis Induced by a New Topoisomerase Inhibitor through the Generation of Hydrogen Peroxide
J. Biol. Chem., August 16, 2002; 277(34): 30684 - 30689.
[Abstract] [Full Text] [PDF]

Home page
 Cancer Res.Home page
J. A. Recio, J. G. Paez, S. Sanders, T. Kawakami, and V. Notario
Partial Depletion of Intracellular ATP Mediates the Stress-Survival Function of the PCPH Oncoprotein
Cancer Res., May 1, 2002; 62(9): 2690 - 2694.
[Abstract] [Full Text] [PDF]

Home page
 Mol. Pharmacol.Home page
M. Huang, P. Kozlowski, M. Collins, Y. Wang, T. A. Haystead, and L. M. Graves
Caspase-Dependent Cleavage of Carbamoyl Phosphate Synthetase II during Apoptosis
Mol. Pharmacol., March 1, 2002; 61(3): 569 - 577.
[Abstract] [Full Text] [PDF]

Home page
 Toxicol PatholHome page
G. M. Williams and M. J. Iatropoulos
Alteration of Liver Cell Function and Proliferation: Differentiation Between Adaptation and Toxicity
Toxicol Pathol, January 1, 2002; 30(1): 41 - 53.
[Abstract] [PDF]

Home page
 Cancer Res.Home page
C. Jiang, Z. Wang, H. Ganther, and J. Lu
Caspases as Key Executors of Methyl Selenium-induced Apoptosis (Anoikis) of DU-145 Prostate Cancer Cells
Cancer Res., April 1, 2001; 61(7): 3062 - 3070.
[Abstract] [Full Text]

This Article
Right arrow Full Text (PDF)
Right arrow Alert me when this article is cited
Right arrow Alert me if a correction is posted
Services
Right arrow Email this article to a friend
Right arrow Similar articles in this journal
Right arrow Similar articles in PubMed
Right arrow Alert me to new issues of the journal
Right arrow Download to citation manager
Right arrow reprints & permissions
Citing Articles
Right arrow Citing Articles via HighWire
Right arrow Citing Articles via Google Scholar
Google Scholar
Right arrow Articles by Martin, D. S.
Right arrow Articles by Koutcher, J. A.
Right arrow Search for Related Content
PubMed
Right arrow PubMed Citation
Right arrow Articles by Martin, D. S.
Right arrow Articles by Koutcher, J. A.

HOME HELP FEEDBACK SUBSCRIPTIONS ARCHIVE SEARCH TABLE OF CONTENTS
Cancer Research Clinical Cancer Research
Cancer Epidemiology Biomarkers & Prevention Molecular Cancer Therapeutics
Molecular Cancer Research Cancer Prevention Research
Cancer Prevention Journals Portal Cancer Reviews Online
Annual Meeting Education Book Meeting Abstracts Online