Investigation of tumor hypoxia using a two-enzyme system for in vitro generation of oxygen deficiency
Radiation Oncologyvolume 6, Article number: 35 (2011)
Oxygen deficiency in tumor tissue is associated with a malign phenotype, characterized by high invasiveness, increased metastatic potential and poor prognosis. Hypoxia chambers are the established standard model for in vitro studies on tumor hypoxia. An enzymatic hypoxia system (GOX/CAT) based on the use of glucose oxidase (GOX) and catalase (CAT) that allows induction of stable hypoxia for in vitro approaches more rapidly and with less operating expense has been introduced recently. Aim of this work is to compare the enzymatic system with the established technique of hypoxia chamber in respect of gene expression, glucose metabolism and radioresistance, prior to its application for in vitro investigation of oxygen deficiency.
Human head and neck squamous cell carcinoma HNO97 cells were incubated under normoxic and hypoxic conditions using both hypoxia chamber and the enzymatic model. Gene expression was investigated using Agilent microarray chips and real time PCR analysis. 14C-fluoro-deoxy-glucose uptake experiments were performed in order to evaluate cellular metabolism. Cell proliferation after photon irradiation was investigated for evaluation of radioresistance under normoxia and hypoxia using both a hypoxia chamber and the enzymatic system.
The microarray analysis revealed a similar trend in the expression of known HIF-1 target genes between the two hypoxia systems for HNO97 cells. Quantitative RT-PCR demonstrated different kinetic patterns in the expression of carbonic anhydrase IX and lysyl oxidase, which might be due to the faster induction of hypoxia by the enzymatic system. 14C-fluoro-deoxy-glucose uptake assays showed a higher glucose metabolism under hypoxic conditions, especially for the enzymatic system. Proliferation experiments after photon irradiation revealed increased survival rates for the enzymatic model compared to hypoxia chamber and normoxia, indicating enhanced resistance to irradiation. While the GOX/CAT system allows independent investigation of hypoxia and oxidative stress, care must be taken to prevent acidification during longer incubation.
The results of our study indicate that the enzymatic model can find application for in vitro investigation of tumor hypoxia, despite limitations that need to be considered in the experimental design.
Reduced oxygen levels are measured in several solid tumors mainly as result of tumor outgrowing the existing vasculature but also as result of structural and functional disturbances of tumor vasculature . In particular, tumor blood vessels that are newly formed during angiogenesis are highly irregular and possess incomplete endothelial linings and basement membranes, as well as arteriovenous shunts, resulting in disturbances of blood flow and oxygen delivery . Tumor hypoxia is associated with a more aggressive neoplastic phenotype, characterized by high invasiveness and increased metastatic potential. Genes with key-role in metastatic processes, such as lysyl oxidase (LOX), met proto-oncogene (MET) and c-X-c chemokine receptor 4 (CXCR4) have been identified to be upregulated under hypoxic conditions [3, 4]. In regard to therapy outcome and prognosis, hypoxic regions within a solid tumor are characterized by increased resistance towards chemotherapy or radiotherapy. In particular, oxygen deficiency upregulates the expression of the multidrug resistance gene (MDR1), leading to efflux of chemotherapeutic drugs . In respect to radiation therapy both chemical and biological mechanisms are found to be important for increased radioresistance. Oxygen deficiency disturbs the radiolysis of H2O leading to reduced production of reactive species that are cytotoxic . Furthermore, hypoxia promotes the activation of the hypoxia inducible factor-1 (HIF-1), a heterodimeric transcription factor that upregulates the expression of genes involved in angiogenesis and tumorigenesis .
The fact that tumor hypoxia is associated with increased therapy resistance and poor prognosis reveals the necessity for extensive and detailed investigation of biological mechanisms associated with oxygen deficiency. The established method for in vitro investigation of tumor hypoxia is the exposure of cultured cells to defined, oxygen deficient gaseous environments. The most common apparatus used for this purpose is the hypoxia chamber. However this approach has critical limitations, mainly in regard to oxygen diffusion and equilibration. In particular, within a hypoxia chamber oxygen reaches the cell surface after a protracted process, including transport in the chamber, passing through the material of the cell culture plate, solubility depended entering the culture medium at the gas-medium interface and diffusion through the medium to the cell surface. Oxygen transport kinetic studies in the past have revealed required time periods of about 30 min for equilibration of pO2 between the gas inside and outside of the culture plate and more than 3 h for equilibration of the pO2 between the medium inside the plate and the gas outside of it .
Recently an alternative way to generate in vitro oxygen-deficient conditions has been evaluated [9, 10]. This system is based on the use of the enzymes glucose oxidase (GOX) and catalase (CAT). Addition of glucose oxidase into the cell culture medium removes oxygen by oxidizing glucose. The reaction leads to generation of hydrogen peroxide, which is then removed by catalase, in order to prevent cytotoxic effects due to accumulation. This enzymatic system was found to induce rapid depletion of oxygen within minutes at a defined rate. Oxygen concentration in the cultured medium is reported to be dependent by two factors: the activity of glucose oxidase and the medium volume. GOX activity has an influence on the depletion rate of oxygen, while medium volume affects the diffusion distance of oxygen from gas-medium interface to the cells. Experiments have revealed that at defined GOX activity and medium volume, controlled oxygen depletion can be achieved and also stably maintained for at least 12-24 h .
Aim of the present work is to investigate the effects of rapidly induced hypoxia on cellular processes using the enzymatic GOX/CAT system in comparison to the established method of hypoxia chamber. Since hypoxia is known to be a feature of human head and neck squamous cell carcinoma , the HNSCC cell line HNO97 was chosen for investigation under normoxic and hypoxic conditions using a hypoxia chamber and the enzymatic model. We focused on three aspects: gene expression, glucose metabolism and radioresistance. Gene expression was investigated using Agilent microarray chip analysis and real time PCR. Cellular glucose metabolism was assessed with 14C-FDG uptake assays and proliferation experiments after photon irradiation were carried out for investigation of hypoxia induced radioresistance. The results of our study indicate that the enzymatic GOX/CAT system is an attractive alternative technique for in vitro investigation of tumor hypoxia.
The human head and neck squamous cell carcinoma cell line HNO97  was cultivated in Dulbecco's Modified Eagle's Medium (DMEM containing 4.5 g/L glucose and 58 ng/L L-glutamine but no sodium pyruvate) supplemented with 10% (v/v) fetal calf serum (Gibco, Invitrogen Life Technologies) at 37°C in a 5% CO2 incubator.
In vitro enzymatic and non-enzymatic hypoxia induction
Hypoxia medium was prepared by diluting glucose oxidase and catalase at a constant 1:10 ratio in cell culture medium (both Sigma cat. No. C3155 and G0543). Enzyme activities of stock solutions were 3 mM/s for GOX and 998 s-1 for CAT. To obtain a defined, stable oxygen concentration of 2% on cell surface stock solutions were diluted by 1:10,000 for GOX and 1:1,000 for CAT. The medium volumes used were 2.5 ml for 6-well plates and 10.63 ml for 10 cm cell culture plates and the cells were incubated at 37°C. Previous experiments using a computer-driven oxygen electrode Oxi 325-B (WTW, Weilheim, Germany) for oxygen measurement have revealed that at those conditions 2% hypoxia was rapidly induced within 15 min and maintained over 24 h . For incubation periods longer than 24 h medium was replaced by pre-equilibrated hypoxic medium to maintain nutrients and substrates such as glucose.
Cells cultivated in 6-well plates or 10 cm cell culture dishes under a layer of exactly 2.5 ml and 10.63 ml cell culture medium respectively were placed in a hypoxia chamber. The chamber was flushed with 2% O2/5% CO2/93% N2 gas mixture for 5 min, sealed and kept at 37°C. For longer incubation periods the chamber was refilled after 24 h to ensure constant oxygen concentrations.
Real time quantitative PCR
Total cellular RNA was isolated from confluent head and neck squamous cell carcinoma HNO97 cells using Trizol (TRIzol Reagent, Invitrogen #15596-018) according to manufacturer instructions. RNA concentration was measured with a NanoDrop spectrophotometer (ND-1000 PeqLab Biotechnologie GmbH, Germany). 500 ng was transcribed into DNA using M-MLV reverse transcriptase, 50 pmol random hexamer and 100 pmol of oligo(dT) primers (Promega, Madison, WI, USA). Quantification of relative mRNA transcript levels of human carbonic anhydrase IX (CA9) and lysyl oxidase (LOX) was performed on a StepOnePlus™ Real-Time PCR System (Applied Biosystems), applying the TaqMan methodology. Normalization was performed using B2 microglobulin (B2M) as endogenous control. Primers were obtained from Applied Biosystems (Foster City, CA, USA).
Gene expression of HNO97 cells under normoxic and hypoxic conditions was investigated using whole human genome microarrays. Total RNA from time points t = 0, and after 24 h incubation under hypoxic conditions (2% O2) using the hypoxia chamber and the GOX/CAT system was investigated. To determine the influence of cell density on gene expression, microarray analysis was also performed for RNA isolated from cells incubated for the same time period (24 h) under normoxic conditions. For bioinformatical-analysis a step-wise approach was applied: Weak signals, below the intensity of spike-in linearity, were excluded, quantile normalization was performed on background-subtracted signal intensities, ratios were calculated by arithmetic mean normalization of control group (t = 0 or normoxia t = 24 h) versus all samples. Afterwards Log2 of ratios was calculated.
Microarray processing and data extraction
Genome-wide expression profiling was carried out using whole human genome 4 × 44 k oligo microarrays (Agilent, G4112F). Linear amplification from 500 ng total RNA and spike-in-controls (Agilent #5188-5282) was performed using the Agilent "Low RNA Input Linear Amplification Kit Plus, one colour" (#5188-5339). During this process the amplified RNA was directly labelled by incorporation of Cy3-labelled CTP. Labelled RNA was purified with "RNeasy" mini spin columns (Qiagen #74104) and 1.65 μg labelled RNA was used for chemical fragmentation and hybridisation (Gene expression hybridization kit, Agilent #5188-5242). Assembly of the gasket/slide-sandwich in the hybridisation chamber (Agilent, #G2534A) was performed according to manufacturer instructions. For hybridisation, slide-sandwiches were rotated at 10 rpm and 65°C for 16 h. Slides were washed 1 min in GE Wash Buffer 1 at RT, 1 min in GE Wash Buffer 2 at RT (Agilent, #5188-5325, 5188-5326) and 30 sec in Acetonitril at RT on a magnetic stirrer. Slides were scanned in an Agilent Microarray Scanner. Data extraction of the resulting array images was performed using the "Feature Extraction" software (Agilent, Version 9.1) and SUMO (Christian Schwager, http://angiogenesis.dkfz.de/oncoexpress/software/sumo/) was used for statistical analysis, two-class t-tests and GO-analysis. Pathway analysis was performed based on information available on cellular signalling processes from a curated database on signalling networks and systems biology package (Metacore, Genego, St Joseph, MI, USA, http://www.genego.com).
After trypsinisation 5 × 104 HNO97 cells were seeded in 6-well plates. Cells were incubated in DMEM + 10% FCS for 24 h. Medium was removed and the cells were incubated for 6 h and 24 h under normoxic and hypoxic conditions (2% O2), using the enzymatic GOX/CAT system and a hypoxia chamber. Subsequently, FDG uptake experiments were performed in glucose-free DMEM medium as described in the literature . In particular, after 30 min of pre-incubation in glucose-free medium, 37 kBq 2-fluoro-2-deoxy-D-[U-14C] glucose (FDG; Amersham-Buchler; specific activity 10.8 GBq/mmol; radioactive concentration 7.4 MBq/ml; radiochemical purity 99.3%) per ml medium and cold FDG were added to a final concentration of 0.1 mM. Cells were incubated for 10 min with radioactive FDG and thereafter the medium was removed and the cells were washed three times with ice-cold PBS. Cells were then lysed on ice with 1M NaOH. The lysates were counted on a scintillation counter. The viable cell number was determined by a Vi-Cell™ XR Cell Viability Analyzer (Beckman Coulter). Radioactive FDG uptake was calculated as % applied dose per 106 cells. The experiment was performed in triplicate and repeated twice.
50,000 human head and neck squamous cell carcinoma HNO97 cells were seeded in 6-well plates and incubated overnight at standard conditions and subsequently for 24 h under normoxia and hypoxia (2% O2) using both the enzymatic GOX/CAT system and a hypoxia chamber. Thereafter, cells were trypsinized and their viability was investigated with automated trypan blue viability assays using a Vi-Cell™ XR Cell Viability Analyzer (Beckman Coulter).
Cell irradiation and proliferation assay
Proliferation assays were performed as described in the literature . 50,000 human head and neck squamous cell carcinoma HNO97 cells were seeded in 6-well plates and incubated overnight at standard conditions. The cells were then incubated for 24 h at normoxic and hypoxic conditions using both the enzymatic GOX/CAT system and a hypoxia chamber. Irradiation with 6 MV X-rays (Mevatron Siemens) at a dose of 4 Gy was performed and further incubation for 72 h at the same conditions as before irradiation was carried out. Thereafter the cells were trypsinized and counted with a Vi-Cell™ XR Cell Viability Analyzer (Beckman Coulter). Non-irradiated cells were incubated at the same conditions. The ratio vital irradiated/non-irradiated cells, which represents the proportion of vital cells after irradiation, compared to the non-irradiated control was calculated.
Statistical analysis of the genomics was performed with SUMO (Christian Schwager, http://angiogenesis.dkfz.de/oncoexpress/software/sumo/) using two-class t-tests. Data of FDG-uptake and cell proliferation assays were analyzed employing the Student t-test. Significance was assumed at p < 0.05.
After 24 h incubation in a hypoxia chamber and with the GOX/CAT system the expression of known and validated HIF-1 target genes as described in the literature  was evaluated for HNO97 cells. The experiments demonstrated a similar trend in the expression of known HIF-1 target genes for both systems (Figure 1). An overview of the expression of known HIF-1 target genes for HNO97 cells is presented in Additional file 1.
In order to identify the strongest regulated genes for HNO97 cells under hypoxia, a 2-class t-test was performed. The 50 strongest regulated genes and the respective p-values for the GOX/CAT system and the hypoxia chamber compared to normoxic cells at 24 h are presented in Figure 2A. Among them 7 genes are known HIF-1 target genes (CA9, PGK1, ALDOC, COL5A1, FN1, VEGF, ENO2), while 4 further genes are described to be associated with hypoxia (AKR1C3, ICAM1, LOXL2, LAMA3).
Differentially regulated genes between the two hypoxic systems in HNO97 cells were identified performing a two-class t-test after normalization against the control chips from the normoxic cells at t = 24 h. The statistical analysis revealed the 50 strongest differentially regulated genes (Figure 2B). Among them only 1 gene was found to be a HIF-1 target (CXCR4).
Functional groups of hypoxia regulated genes for both systems were identified by assigning them to biological function GO-terms. The most probably regulated GO-Term was Glycolysis (p = 4 × E-5), which is shown in Figure 3.
In addition to microarray analysis (Additional file 1), quantification of the tumor hypoxia regulated genes CA9 and LOX was performed with real time PCR. To evaluate the gene expression under hypoxic conditions over time, HNO97 cells were incubated for time periods of 4 h, 8 h and 24 h under normoxic conditions, in the hypoxia chamber and with the GOX/CAT system. The RT-PCR experiments demonstrated an upregulation of the tumor hypoxia dependent genes for both systems (p < 0.05). However, time kinetic of the gene expression was different between the slow hypoxia chamber and the rapid hypoxia GOX/CAT system. In particular, the highest level of CA9 and LOX expression was shown at 8 h incubation for the enzymatic system and then decreased, while a continuous increase over time for the incubation period was identified for the hypoxia chamber (Figure 4).
Fluorodeoxyglucose (FDG) uptake experiments were carried out in order to evaluate the influence of hypoxia in the metabolic activity of HNO97 cells. For these experiments cells were cultivated under normoxia or hypoxia (2% O2) for 6 h and 24 h and subsequently radioactive FGD was shortly applied on the cells and the uptake was determined. These studies demonstrated an enhanced FDG uptake under hypoxia. After 6 h cultivation the FDG uptake was significantly increased for the GOX/CAT system (p < 0.05). In regard to the hypoxia chamber, only a slight increase was noticed compared to normoxia (Table 1). After 24 h cultivation a significant FDG uptake enhancement was noticed for both hypoxic systems compared to normoxia (p < 0.05). Still, the enhancement of FDG uptake was higher for the rapid hypoxia inducing enzymatic model (p < 0.05) compared to the slower hypoxia inducing chamber (Figure 5). The ratios of FDG uptake under hypoxia to FDG uptake under normoxia are presented for both hypoxia systems in Table 1.
Cell viability was investigated with a Vi-Cell™ XR Cell Viability Analyzer (Beckman Coulter) to determine whether hypoxia at the applied conditions might cause cell death. Cell number evaluation after 24 h cultivation using GOX/CAT and a hypoxia chamber showed absolute cell numbers of about 70% and 90% of the absolute cell number after 24 h cultivation under normoxia. Trypan blue analysis revealed that hypoxia did not induce cell death at the applied conditions. In particular, no significant difference was noticed in the percentage of unvital cells (5-10%) for both normoxia and hypoxia using GOX/CAT or chamber. Furthermore, microscopy studies showed that the cells were still attached and morphologically intact under the hypoxic conditions used (data not shown).
Cell proliferation after photon irradiation
Proliferation of HNO97 cells was investigated for normoxia and hypoxia after photon irradiation at a single dose of 4 Gy. Vital cell number was measured and the ratio vital irradiated/non-irradiated cells, was determined. This ratio represents the proportion of vital cells after irradiation compared to the non-irradiated control. The proliferation assays revealed higher ratios when HNO97 cells were incubated under hypoxic conditions (p < 0.05), indicating an enhanced cell resistance to the applied radiation dose. This ratio was only slightly enhanced for the slow-onset hypoxia chamber system but was higher for the enzymatic GOX/CAT system (p < 0.05) (Figure 6).
To determine whether different cell confluences, as result of different cell growth rates under normoxia and hypoxia, had an influence on irradiation outcome, proliferation experiments after photon irradiation with 4 Gy were performed for various cell confluences under normoxia. These experiments revealed no significant differences in irradiation outcome within the cell number range that was measured for normoxia, hypoxia chamber and GOX/CAT (50,000 to 200,000 cells) at the time of irradiation (Additional file 2).
The microenviroment within a solid tumor has an extensive influence on the outcome of cancer treatment and the prognosis of the disease. Tumor hypoxia affects the behaviour of tumor cells and is associated with poor prognosis and reduced overall survival . This fact reveals the need for a detailed study of biological effects under reduced oxygen levels. The most common technique used to investigate in vitro tumor hypoxia is the hypoxia chamber. However, this approach has limitations. The method requires special technical equipment while it has been shown that it leads to a slow onset of hypoxia that might influence the correlation between changes in oxygen concentration and kinetic of hypoxia dependent biological events.
An alternative to hypoxia chamber represents the enzymatic GOX/CAT system, which has been shown to rapidly induce in vitro hypoxia. The GOX/CAT system has been employed in the past in various studies. In particular, Baumann et al. have applied the enzymatic system for investigation of the effects of the hypoxia-targeted prodrug KS119 [9, 17]. Furthermore, Zitta et al. used GOX/CAT for rapidly induction of hypoxia and investigated the influence of mild hypothermia and postconditioning with catalase on hypoxia-mediated cell damage , as well as the potential cytoprotective properties of different sevoflurane conditioning strategies on a human neuronal cell culture model . In addition, Owegi et al. applied the GOX/CAT technique to test macrophage activity under various O2 and H2O2 concentrations, as presented under infection conditions . All these studies have demonstrated a rapid decrease of oxygen concentration using glucose oxidase and catalase but provided only limited comparisons to the established hypoxia chamber technique. Therefore, in the present study we evaluated the enzymatic GOX/CAT system in direct comparison to the established hypoxia chamber technique for investigation of different biological events, including gene expression, glucose uptake and radioresistance at a defined O2 concentration.
The conditions for in vitro generation of hypoxia at a level of 2% were carefully chosen in concert with the results of previous studies. In particular, evaluation of oxygen concentration using a computer-driven oxygen electrode revealed that at the conditions used for our experiments 2% hypoxia was rapidly induced within 15 min and maintained over 24 h . Since oxygen transport studies using hypoxia chambers have revealed time periods of more than 3 h for equilibration of pO2 between the medium inside the plate and the gas outside of it, which even accelerated in the presence of cells , evaluation of both systems was performed after 24 h cell cultivation under hypoxic conditions to ensure that the observed biological events are not a result of differences in the oxygenation level. We further chose for our investigation a head and neck squamous cell carcinoma (HNSCC) cell line because there is strong evidence that hypoxia is an important microenvironment factor, which influences the response of HNSCC to therapy  and because the role of low oxygen tension has been extensively investigated for this cancer entity both in preclinical and in clinical studies [22, 23].
Our experiments demonstrated comparable trends for both systems in regard to gene expression, glucose uptake and resistance towards radiation therapy. In particular, investigation of hypoxia related genes using microarray chip analysis in our study revealed a similar regulation trend for most known HIF-1 target genes for both the rapid enzymatic GOX/CAT system and the hypoxia chamber after 24 h of hypoxia (Figure 1). The expression of prominent hypoxia dependent genes, such as carbonic anhydrase IX (CA9) and lysyl oxidase (LOX) was additionally to microarray analysis quantified by real time PCR. These genes were chosen for analysis not only because it is known that they are hypoxia regulated, but also because various studies have reported prognostic values for them in head and neck squamous cell carcinoma [24, 25]. Microarray analysis in our study indicated CA9 and LOX activation both in the chamber and the enzymatic system after 24 h, while CA9 showed stronger activation than LOX. Quantification through real time PCR demonstrated different kinetic patterns between the two hypoxia systems (Figure 4). Particularly, although both genes were upregulated under hypoxic conditions the upregulation peak was reached earlier for the rapid enzymatic GOX/CAT system and decreased thereafter, compared to the hypoxia chamber that showed a continuous increase of gene expression over 24 h. Our results are in concert with the results of previous studies using the GOX/CAT system . Millonig et al. have shown that a fast onset of hypoxia using the enzymatic system leads to rapid induction of HIF-1 that later disappears although the cells remain under stable hypoxia. In contrast, cell exposure to the same oxygen concentration using a conventional hypoxia chamber causes a late onset and continuous upregulation of HIF-1 over a time period of 24 h. These results led the authors to the conclusion that HIF-1 responds rather to oxygen decrements than to absolute hypoxia, a hypothesis that might also explain the different kinetic patterns of the HIF-1-target genes CA9 and LOX as demonstrated in our study.
In regard to glucose metabolism, uptake experiments of fluorodeoxyglucose (FDG) revealed an enhanced cellular uptake for both the enzymatic and the chamber system (Figure 5), which increased with time progression (Table 1). This result is expected, since it is known that hypoxia is associated with a reprogrammed cellular metabolism, characterized by enhanced uptake of glucose for use as anabolic and catabolic substrate. The enhanced FDG uptake is supported by a HIF-1 dependent activation of the transcription of SLC2A1 and SLC2A3 genes, which encode the glucose transporters GLUT1 and GLUT3 respectively. Furthermore, HIF-1 activates the transcription of the HK1 and HK2 genes, which encode for hexokinase, an enzyme that phosphorylates FDG and represents the first enzyme of the Embden-Meyerhoff (glycolytic) pathway [26, 27]. The role of HIF-1 in further metabolisation of glucose has been extensively investigated in previous studies. In particular, it has been shown that glycolytic enzymes which metabolize glucose to pyruvate, and lactate dehydrogenase A (LDHA) which further converts pyruvate to lactate are regulated by HIF-1, promoting ATP production through increased anaerobic glycolysis under hypoxic conditions . The results of our study demonstrate that the new enzymatic GOX/CAT system affects glucose metabolism in a similar trend like the established hypoxia chamber. FDG uptake was increased for both systems, result that is in concert with the microarray analysis, which shows an upregulation of genes involved in glucose metabolism, such as SLC2A1, SLC2A3, HK1, HK2 and LDHA. The slower increase of FDG uptake for the hypoxia chamber, compared to GOX/CAT (Table 1) might be explained by different kinetics in the expression of HIF-1 target genes that are involved in glucose metabolism, considering the fact that further HIF-1 target genes, such as CA9 and LOX showed different expression kinetics for the two systems.
In regard to glucose metabolism, assignment of gene expression results to biological function gene ontology terms (GO-terms), demonstrated glycolysis to be the most probably regulated GO-term for both systems (Figure 3). This is expected since glycolysis is known to be the preferred route for energy production under conditions of oxygen deficiency. Although our results provide strong indications of glycolytic metabolism, further investigation of the ratio between lactate production and glucose consumption is needed in order to assess the balance between glycolytic and oxidative metabolism under normoxia and hypoxia using the GOX/CAT system. This is important, considering the fact that cancer cells are known to use glycolysis even under normoxic conditions. Since glycolysis can produce ATP at higher rates than oxidative phosphorylation  and tumor cells require fast energy production in order to support cell growth and survival, metabolic alterations in favour of glycolysis is noticed even under normoxia , demonstrating the complexity of pathways and mechanisms in respect to microenvironment adaptation of tumor cells.
The enzymatic GOX/CAT system has however a critical limitation that needs to be considered in experiments investigating glucose metabolism. Glucose oxidase (GOX) does not only consume oxygen but also leads to depletion of glucose in the incubation medium. Previous studies investigating in vitro FDG uptake in various cell lines have revealed that hypoglycemic conditions lead to an increased FDG uptake [31, 32]. Furthermore, it has been shown that the enhanced transport activity caused by hypoglycemia is attributed to an increased expression of GLUT1 in the cell membrane . Therefore, the GOX mediated glucose depletion might bias the results of metabolic experiments. The substrate consumption at various settings of the GOX/CAT system has been extensively evaluated . Under our conditions, hypoxia could be stably maintained for about 24 h without replacing the medium and reagents, leading to a glucose decrease of about 10% . For comparison, 5% equals the 24-hour glucose consumption of about 90 million exponentially growing tumor cells .
Subphysiologic levels of oxygen in the tumor lead to an up to 3-fold increase of resistance against antineoplastic strategies, such as radiation therapy . The enhanced radioresistance is explained through a reduced production of cytotoxic reactive species and promotion of the upregulation of genes that protect the cells from irradiation . Within our study we performed proliferation experiments after irradiation of the cells in order to investigate whether the enzymatic GOX/CAT system could be used for in vitro investigation of hypoxia related radioresistance. The comparison with the established hypoxia chamber revealed that at O2 concentration of 2% only a slight resistance increase was noticed for the hypoxia chamber system, while the GOX/CAT system showed a higher resistance to photon irradiation (Figure 6). The enhanced radioresistance for the rapid hypoxic strategy could be explained by an increased growth arrest in the G0/G1 phase of the cell cycle. It has been shown in the past that one of the genes that promote growth arrest in the G0/G1 phase via upregulation of p21 is heme oxygenase 1 (HMOX1) . Our gene expression analysis revealed a strongly increased expression of HMOX1 for the GOX/CAT system compared to the hypoxia chamber (Log2 of 3.5 and 0.2, respectively), result that offers a possible explanation for the enhanced cytoprotection that needs to be further investigated.
The hypothesis of growth arrest through rapid hypoxia is supported by the results of viability experiments irrespective of irradiation. These experiments showed lower cell numbers for the hypoxic systems compared to normoxia. Trypan blue and microscopy analysis revealed however that the reduced cell number was not attributed to cell death. Our results might be explained by a reduced cell division and DNA synthesis, which has been described in previous studies using the enzymatic model .
The GOX/CAT system has some limitations. Besides the fact that GOX causes glucose depletion and therefore the results might be affected by substrate deprivation, the activity of GOX also leads to the production of D-gluconolactone, which may cause culture medium acidification. pH measurement during our studies with HNO97 cells revealed no significant acidification of the DMEM medium for the investigated time period of 24 h. However, using the GOX/CAT system for hypoxia induction on human umbilical vein endothelial cells (HUVEC) a rapid pH decrease to a level of about 4.0-4.5 was noticed, leading to RNA degradation and cell death (data not shown). The extracellular pH of malignant tumors is known to be acidic, within a range of 6.5 to 7.0, as a consequence of increased glucose metabolism and poor perfusion , promoting tumor cell invasion via several matrix remodeling systems, including metalloproteinases, lysosomal proteases and hyaluronidase [40, 41]. However, the strong acidosis measured on HUVEC cells using the GOX/CAT system, can not only be attributed to physiologically induced acidocis. A possible explanation is a low buffer capacity of the HUVEC cell culture medium, which needs to be considered in the design of experiments using the GOX/CAT system. In order to minimize substrate depletion and gluconolactone production two strategies can be applied for incubation periods longer than 24 h. The first strategy is the replacement of the incubation medium by fresh, preequilibrated medium and the second is the use of larger volumes of medium, which will in turn increase the time to reach stable hypoxia .
Finally, it should be mentioned that the GOX/CAT system allows the additional generation and control of hydrogen peroxide independently of the degree of hypoxia [34, 42]. Since reactive oxygen species play an important role during tumor growth and radiation therapy of tumors, this option may be highly interesting when studying the role of transcription factors such as HIF-1 that are both responsive to hypoxia but also reactive oxygen species.
In conclusion, the results of our study indicate that the GOX/CAT system might be a useful tool for the in vitro investigation of tumor hypoxia. In comparison to the established hypoxia chamber techniques, the GOX/CAT approach can induce hypoxia rapidly and in a controlled manner, while it is inexpensive and does not require technical equipment. Despite limitations which should be considered in the experimental design, the enzymatic system represents an attractive and valuable alternative for studying biological events associated with tumor hypoxia that needs to be further investigated.
Milani M, Harris AL: Targeting tumour hypoxia in breast cancer. Eur J Cancer 2008, 44: 2766-2773. 10.1016/j.ejca.2008.09.025
Brown JM: Exploiting the hypoxic cancer cell: mechanisms and therapeutic strategies. Mol Med Today 2000, 6: 157-162. 10.1016/S1357-4310(00)01677-4
Erler JT, Bennewith KL, Nicolau M, Dornhöfer N, Kong C, Le QT, Chi JT, Jeffrey SS, Giaccia AJ: Lysyl oxidase is essential for hypoxia induced metastasis. Nature 2006, 440: 1222-1226. 10.1038/nature04695
Pennacchietti S, Michieli P, Galluzzo M, Mazzone M, Giordano S, Comoglio PM: Hypoxia promotes invasive growth by transcriptional activation of the met protooncogene. Cancer Cell 2003, 3: 347-361. 10.1016/S1535-6108(03)00085-0
Comerford KM, Wallace TJ, Karhausen J, Louis NA, Montalto MC, Colgan SP: Hypoxia-inducible factor-1-dependent regulation of the multidrug resistance (MDR1) gene. Cancer Res 2002, 62: 3387-3394.
Gray LH, Conger AD, Ebert M, Hornsey S, Scott OC: The concentration of oxygen dissolved in tissues at the time of irradiation as a factor in radiotherapy. Br J Radiol 1953, 26: 638-648. 10.1259/0007-1285-26-312-638
Carmeliet P, Dor Y, Herbert JM, Fukumura D, Brusselmans K, Dewerchin M, Neeman M, Bono F, Abramovitch R, Maxwell P, Koch CJ, Ratcliffe P, Moons L, Jain RK, Collen D, Keshert E: Role of HIF-1alpha in hypoxia-mediated apoptosis, cell proliferation and tumour angiogenesis. Nature 1998, 394: 485-490. 10.1038/28867
Allen CB, Schneider KB, White CW: Limitations to oxygen diffusion and equilibration in in vitro cell exposure systems in hyperoxia and hypoxia. Am J Physiol Lung Cell Mol Physiol 2001, 281: 1021-1027.
Baumann RP, Penketh PG, Seow HA, Shyam K, Sartorelli AC: Generation of oxygen deficiency in cell culture using a two-enzyme system to evaluate agents targeting hypoxic tumor cells. Radiat Res 2008, 170: 651-660. 10.1667/RR1431.1
Millonig G, Hegedüsch S, Becker L, Seitz HK, Schuppan D, Mueller S: Hypoxia-inducible factor 1 alpha under rapid enzymatic hypoxia: cells sense decrements of oxygen but not hypoxia per se. Free Radic Biol Med 2009, 46: 182-191. 10.1016/j.freeradbiomed.2008.09.043
Troost EG, Schinagl DA, Bussink J, Boerman OC, van der Kogel AJ, Oyen WJ, Kaanders JH: Innovations in radiotherapy planning of head and neck cancers: role of PET. J Nucl Med 2010, 51: 66-76. 10.2967/jnumed.108.061499
Ninck S, Reisser C, Dyckhoff G, Helmke B, Bauer H, Herold-Mende C: Expression profiles of angiogenic growth factors in squamous cell carcinomas of the head and neck. Int J Cancer 2003, 106: 34-44. 10.1002/ijc.11188
Haberkorn U, Altmann A, Kamencic H, Morr I, Traut U, Henze M, Jiang S, Metz J, Kinscherf R: Glucose transport and apoptosis after gene therapy with HSV thymidine kinase. Eur J Nucl Med 2001, 28: 1690-1696. 10.1007/s002590100644
Bischof M, Abdollahi A, Gong P, Stoffregen C, Lipson KE, Debus JU, Weber KJ, Huber PE: Triple combination of irradiation, chemotherapy (pemetrexed), and VEGFR inhibition (SU5416) in human endothelial and tumor cells. Int J Radiat Oncol Biol Phys 2004, 60: 1220-1232. 10.1016/j.ijrobp.2004.07.689
Benita Y, Kikuchi H, Smith AD, Zhang MQ, Chung DC, Xavier RJ: An integrative genomics approach identifies Hypoxia Inducible Factor-1 (HIF-1)-target genes that form the core response to hypoxia. Nucleic Acids Res 2009, 37: 4587-4602. 10.1093/nar/gkp425
Demir R, Naschberger L, Demir I, Melling N, Dimmler A, Papadopoulus T, Sturzl M, Klein P, Hohenberger W: Hypoxia generates a more invasive phenotype of tumour cells: an in vivo experimental setup based on the chorioallantoic membrane. Pathol Oncol Res 2009, 15: 417-422. 10.1007/s12253-008-9140-y
Baumann RP, Penketh PG, Ishiguro K, Shyam K, Zhu YL, Sartorelli AC: Reductive activation of the prodrug 1,2-bis(methylsulfonyl)-1-(2-chloroethyl)-2-[[1-(4-nitrophenyl)ethoxy]carbonyl]hydrazine (KS119) selectively occurs in oxygen-deficient cells and overcomes O(6)-alkylguanine-DNA alkyltransferase mediated KS119 tumor cell resistance. Biochem Pharmacol 2010, 79: 1553-1561. 10.1016/j.bcp.2009.12.004
Zitta K, Meybohm P, Bein B, Rodde C, Steinfath M, Scholz J, Albrecht M: Hypoxia-induced cell damage is reduced by mild hypothermia and postconditioning with catalase in-vitro: application of an enzyme based oxygen deficiency system. Eur J Pharmacol 2010, 628: 11-18. 10.1016/j.ejphar.2009.11.023
Zitta K, Meybohm P, Bein B, Ohnesorge H, Steinfath M, Scholz J, Albrecht M: Cytoprotective effects of the volatile anesthetic sevoflurane are highly dependent on timing and duration of sevoflurane conditioning: findings from a human, in-vitro hypoxia model. Eur J Pharmacol 2010, 645: 39-46. 10.1016/j.ejphar.2010.07.017
Owegi HO, Egot-Lemaire S, Waite LR, Waite GN: Macrophage activity in response to steady-state oxygen and hydrogen peroxide concentration- biomed 2010. Biomed Sci Instrum 2010, 46: 57-62.
Silva P, Homer JJ, Slevin NJ, Musgrove BT, Sloan P, Price P, West CM: Clinical and biological factors affecting response to radiotherapy in patients with head and neck cancer: a review. Clin Otolaryngol 2007, 32: 337-345. 10.1111/j.1749-4486.2007.01544.x
Sørensen BS, Horsman MR, Vorum H, Honoré B, Overgaard J, Alsner J: Proteins upregulated by mild and severe hypoxia in squamous cell carcinomas in vitro identified by proteomics. Radiother Oncol 2009, 92: 443-449.
Rischin D, Hicks RJ, Fisher R, Binns D, Corry J, Porceddu S, Peters LJ, Trans-Tasman Radiation Oncology Group Study 98.02: Prognostic significance of [18F]-misonidazole positron emission tomography-detected tumor hypoxia in patients with advanced head and neck cancer randomly assigned to chemoradiation with or without tirapazamine: a substudy of Trans-Tasman Radiation Oncology Group Study 98.02. J Clin Oncol 2006, 24: 2098-2104. 10.1200/JCO.2005.05.2878
De Schutter H, Landuyt W, Verbeken E, Goethals L, Hermans R, Nuyts S: The prognostic value of the hypoxia markers CA IX and GLUT 1 and the cytokines VEGF and IL 6 in head and neck squamous cell carcinoma treated by radiotherapy +/- chemotherapy. BMC Cancer 2005, 5: 42. 10.1186/1471-2407-5-42
Le QT, Harris J, Magliocco AM, Kong CS, Diaz R, Shin B, Cao H, Trotti A, Erler JT, Chung CH, Dicker A, Pajak TF, Giaccia AJ, Ang KK: Validation of lysyl oxidase as a prognostic marker for metastasis and survival in head and neck squamous cell carcinoma: Radiation Therapy Oncology Group trial 90-03. J Clin Oncol 2009, 27: 4281-4286. 10.1200/JCO.2008.20.6003
Semenza GL: HIF-1: upstream and downstream of cancer metabolism. Curr Opin Genet Dev 2010, 20: 51-56. 10.1016/j.gde.2009.10.009
Iyer NV, Kotch LE, Agani F, Leung SW, Laughner E, Wenger RH, Gassmann M, Gearhart JD, Lawler AM, Yu AY, Semenza GL: Cellular and developmental control of O2 homeostasis by hypoxia-inducible factor 1 alpha. Genes Dev 1998, 12: 149-162. 10.1101/gad.12.2.149
Vander Heiden MG, Cantley LC, Thompson CB: Understanding the Warburg effect: the metabolic requirements of cell proliferation. Science 2009, 324: 1029-1033. 10.1126/science.1160809
Pfeiffer T, Schuster S, Bonhoeffer S: Cooperation and competition in the evolution of ATP-producing pathways. Science 2001, 292: 504-507. 10.1126/science.1058079
Vousden KH, Ryan KM: p53 and metabolism. Nat Rev Cancer 2009, 9: 691-700. 10.1038/nrc2715
Maschauer S, Prante O, Hoffmann M, Deichen JT, Kuwert T: Characterization of 18F-FDG uptake in human endothelial cells in vitro. J Nucl Med 2004, 45: 455-460.
Gaposchkin CG, Garcia-Diaz JF: Modulation of cultured brain, adrenal, and aortic endothelial cell glucose transport. Biochim Biophys Acta 1996, 1285: 255-266. 10.1016/S0005-2736(96)00172-1
Regina A, Roux F, Revest PA: Glucose transport in immortalized rat brain capillary endothelial cells in vitro: transport activity and GLUT1 expression. Biochim Biophys Acta 1997, 1335: 135-143.
Mueller S, Millonig G, Waite GN: The GOX/CAT system: a novel enzymatic method to independently control hydrogen peroxide and hypoxia in cell culture. Adv Med Sci 2009, 54: 121-135. 10.2478/v10039-009-0042-3
Freyer JP, Sutherland RM: A reduction in the in situ rates of oxygen and glucose consumption of cells in EMT6/Ro spheroids during growth. J Cell Physiol 1985, 124: 516-524. 10.1002/jcp.1041240323
Bussink J, Kaanders JH, van der Kogel AJ: Tumor hypoxia at the micro-regional level: clinical relevance and predictive value of exogenous and endogenous hypoxic cell markers. Radiother Oncol 2003, 67: 3-15. 10.1016/S0167-8140(03)00011-2
Jubb AM, Pham TQ, Hanby AM, Frantz GD, Peale FV, Wu TD, Koeppen HW, Hillan KJ: Expression of vascular endothelial growth factor, hypoxia inducible factor 1alpha, and carbonic anhydrase IX in human tumours. J Clin Pathol 2004, 57: 504-512. 10.1136/jcp.2003.012963
Inguaggiato P, Gonzalez-Michaca L, Croatt AJ, Haggard JJ, Alam J, Nath KA: Cellular overexpression of heme oxygenase-1 up-regulates p21 and confers resistance to apoptosis. Kidney Int 2001, 60: 2181-2191. 10.1046/j.1523-1755.2001.00046.x
Griffiths JR: Are cancer cells acidic? Br J Cancer 1991, 64: 425-427. 10.1038/bjc.1991.326
Robey IF, Baggett BK, Kirkpatrick ND, Roe DJ, Dosescu J, Sloane BF, Hashim AI, Morse DL, Raghunand N, Gatenby RA, Gillies RJ: Bicarbonate increases tumor pH and inhibits spontaneous metastases. Cancer Res 2009, 69: 2260-2268. 10.1158/0008-5472.CAN-07-5575
Ferreira LM: Cancer metabolism: the Warburg effect today. Exp Mol Pathol 2010, 89: 372-380. 10.1016/j.yexmp.2010.08.006
Andriopoulos B, Hegedüsch S, Mangin J, Riedel HD, Hebling U, Wang J, Pantopoulos K, Mueller S: Sustained hydrogen peroxide induces iron uptake by transferrin receptor-1 independent of the iron regulatory protein/iron responsive element network. J Biol Chem 2007, 282: 20301-20308. 10.1074/jbc.M702463200
Acknowledgements and Funding
The authors would like to thank Sylvia Trinh, Claudia Rittmüller and Barbara Schwager for their excellent technical support. Vasileios Askoxylakis has been supported by the Post-Doc Program of the Medical Faculty of the University of Heidelberg. Gunda Millonig has been supported by the Olympia-Morata-Fellowship of the Heidelberg Medical School.
The authors declare that they have no competing interests.
VA and GM made substantial contributions to conception and design of the study, drafted the manuscript and gave approval of the final version. VA, GM, UW, CS and SR were involved in data analysis and data interpretation. AA, UH, JD, SM and PEH were involved in critically revising the manuscript for important intellectual content and gave approval of the final version. All authors have read and approved the final manuscript.