CNS progenitor cells and oligodendrocytes are targets of chemotherapeutic agents in vitro and in vivo
© Dietrich et al.. 2006
Received: 27 March 2006
Accepted: 6 October 2006
Published: 30 November 2006
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© Dietrich et al.. 2006
Received: 27 March 2006
Accepted: 6 October 2006
Published: 30 November 2006
Chemotherapy in cancer patients can be associated with serious short- and long-term adverse neurological effects, such as leukoencephalopathy and cognitive impairment, even when therapy is delivered systemically. The underlying cellular basis for these adverse effects is poorly understood.
We found that three mainstream chemotherapeutic agents – carmustine (BCNU), cisplatin, and cytosine arabinoside (cytarabine), representing two DNA cross-linking agents and an antimetabolite, respectively – applied at clinically relevant exposure levels to cultured cells are more toxic for the progenitor cells of the CNS and for nondividing oligodendrocytes than they are for multiple cancer cell lines. Enhancement of cell death and suppression of cell division were seen in vitro and in vivo. When administered systemically in mice, these chemotherapeutic agents were associated with increased cell death and decreased cell division in the subventricular zone, in the dentate gyrus of the hippocampus and in the corpus callosum of the CNS. In some cases, cell division was reduced, and cell death increased, for weeks after drug administration ended.
Identifying neural populations at risk during any cancer treatment is of great importance in developing means of reducing neurotoxicity and preserving quality of life in long-term survivors. Thus, as well as providing possible explanations for the adverse neurological effects of systemic chemotherapy, the strong correlations between our in vitro and in vivo analyses indicate that the same approaches we used to identify the reported toxicities can also provide rapid in vitro screens for analyzing new therapies and discovering means of achieving selective protection or targeted killing.
One of the disturbing findings to emerge from studies on cancer survivors is the frequency with which chemotherapy is associated with adverse neurological sequelae. Adverse neurological effects associated with treatment of both childhood and adult cancers range from abnormalities detected by CNS imaging (for example, damage to white matter) [1–3] to clinical symptoms. Neurological complications observed as a consequence of chemotherapy include leukoencephalopathy, seizures, cerebral infarctions, and cognitive impairment [4–10].
While it is perhaps not surprising that neurotoxicity occurs after localized delivery of chemotherapeutic agents to the CNS, it is increasingly apparent that this is also a substantial problem associated with the systemic delivery of these agents for treatment of non-CNS tumors [11–18]. For example, current data suggest that 18% of all breast cancer patients receiving standard-dose chemotherapy show cognitive defects on post-treatment evaluation , and such problems were reported in more than 30% of patients examined two years after treatment with high-dose chemotherapy [7, 8], a greater than eightfold increase over the frequency of such changes in control individuals. Even these numbers may be underestimates of the frequency of adverse neurological sequelae in association with aggressive chemotherapy, as two longitudinal studies on breast cancer patients treated with high-dose chemotherapy with carmustine (BCNU), cisplatin, and cyclophosphamide, and evaluated using magnetic resonance imaging and proton spectroscopy, have shown that changes in white matter in the CNS induced by the treatment could occur in up to 70% of individuals, usually with a delayed onset of several months after treatment [1, 2]. Even if examination of all cancers were to lower the frequency of these problems to 25% of the lower estimates (that is, around 4.5% of patients receiving low-dose therapy and 7.5% of patients receiving high-dose chemotherapy) the prevalence of cancer in the world's populations means that the total number of individuals for whom adverse neurological changes are associated with cancer treatment is as great as for many of the more widely recognized neurological syndromes.
Despite the clear evidence of the neurotoxicity of at least some forms of chemotherapy, studies on the effects of chemotherapeutic compounds on brain cells are surprisingly rare. For example, it is known that application of methotrexate directly into the ventricles of the brain is associated with ventricular dilation, edema, and the visible destruction of the ependymal cell layer lining the ventricles and the surrounding brain tissue . Application of cytosine arabinoside (cytarabine) onto the surface of the brain is also associated with adverse effects on the dividing cells of the subventricular zone of the CNS . In vitro studies  have also shown that oligodendrocytes are vulnerable to killing by carmustine (BCNU, an alkylating agent used in the treatment of brain tumors, myeloma, and both Hodgkin and non-Hodgkin lymphoma) at doses that would be routinely achieved during treatment. In general, however, relatively little is known about the effects of chemotherapeutic agents on the cells of the CNS, in striking contrast to the extensive investigations on the effects of irradiation on the brain.
To investigate the biological basis of the adverse neurological consequences of chemotherapy, we posed the following questions. Which cells are vulnerable? Is vulnerability restricted to dividing cells? Does toxicity reflect a direct action of chemotherapeutic agents on defined neural populations? How does the sensitivity of primary neural cells compare with that of cancer cells? What are the in vivo effects of chemotherapy on the dividing populations of the CNS? Do chemotherapeutic agents with different modes of action target the same or different populations of normal cells?
One of the unexpected findings to emerge from our studies was that the vulnerability of CNS cells to BCNU and cisplatin was not restricted to rapidly dividing cells, as nondividing oligodendrocytes were as sensitive as neural progenitors to BCNU and cisplatin, consistent with our previous studies on vulnerability of oligodendrocytes to BCNU . Thus, contrary to the widely held view that the toxicity of chemotherapeutic agents is primarily directed against dividing cells, the ability of BCNU and cisplatin to damage normal cell types in the CNS was not limited to rapidly dividing progenitors. Moreover, cell division by itself was not sufficient to confer vulnerability, as rapidly dividing NSCs were more resistant than progenitor cells. Of all the CNS cell types examined, only astrocytes were as resistant as cancer cells. Thus, the major targets of cisplatin and BCNU toxicity appear to be lineage-restricted progenitor cells and nondividing oligodendrocytes.
Normal progenitor cell function also requires cell division, both during development and for purposes of repair. For O-2A/OPCs, where division can be followed over several days in sensitive clonal assays, it is known that agents that can be cytotoxic at high concentrations will induce cessation of division and induction of differentiation when applied at sub-lethal dosages . We therefore asked whether sub-lethal concentrations of cisplatin and BCNU compromised progenitor cell proliferation. These assays were conducted on O-2A/OPCs in order to benefit from the ability to examine proliferation and differentation at the clonal level [41–43].
Cisplatin (5 mg/kg i.p., days 1, 3, and 5) was similar to BCNU in its effects on the DG, and was associated with a prolonged two- to threefold increase in the number of TUNEL+ cells, persisting at least 42 days, compared with sham-injected control animals. In contrast to BCNU, however, cisplatin was associated with only a modest increase in the number of TUNEL+ cells in the CC at 10 days post-treatment (Figure 5), and with no significant increases in apoptotic cells in the SVZ.
To determine whether acute treatment with chemotherapy has the same cellular targets in vivo as in vitro, we combined the TUNEL assay with labeling with cell-type specific antibodies, and analyzed individual cells by confocal microscopy. In order to focus on the immediate targets of the chemotherapy, analysis was conducted in animals sacrificed 1 day after the completion of BCNU treatment.
We also examined the incorporation of bromodeoxyuridine (BrdU) into regions of the CNS in which cell division occurs in adult animals. Such division is highly restricted in the adult CNS, occurring only in particular regions and/or cell types. The SVZ is known to contain dividing cells and represents the major germinal zone in the CNS [48–51]. The hippocampus is also a region of continued cell generation in the adult CNS, with the majority of dividing cells appearing to be neuronal precursor cells [52, 53]. White matter tracts also contain dividing cells that have been characterized as an adult-specific population of O-2A/OPCs. Although in vitro studies have shown that such cells may have long cell-cycle times, dividing in vitro over an average period of 65 hours instead of the 18-hour cell cycle displayed by O-2A/OPCs isolated from young postnatal rats [54, 55], their frequency in the adult CNS is such that they actually appear to be the major dividing cell type in this tissue [56, 57].
BCNU affects different neural progenitor cell populations equally in vivo
38 ± 5
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14 ± 11
Treatment with three injections of cisplatin was also associated with reduced BrdU incorporation in the SVZ, DG, and CC when examined 1 day after the final injection (Figure 8b). In contrast to the effects of BCNU, however, the number of cells incorporating BrdU returned to normal levels in the DG and SVZ 6 weeks after treatment. Only in the CC was the number of BrdU+ cells still reduced at this late time point.
To determine whether the effects seen so far were specific for DNA crosslinking agents, we extended our studies to include the antimetabolite cytarabine, which is commonly used in treating leukemia and lymphomas, and also has been associated with adverse neurological effects [25, 62].
Like cisplatin and BCNU, cytarabine toxicity was not limited to dividing cells, nor did it affect all dividing populations. Treatment for 24 hours with 0.1 μM of cytarabine induced a 2.4 ± 0.06-fold increase in the percentage of apoptotic TUNEL+ oligodendrocytes, and treatment with 2 μM cytarabine for 24 hours killed 82.4 ± 5.8% of oligodendrocytes (data not shown). As these cells were not dividing in the culture conditions used, the toxicity of cytarabine also extends beyond division-dependent effects. Also as with cisplatin and BCNU, purified astrocytes and NSCs (which were dividing rapidly in the culture conditions used) were less sensitive to the effects of cytarabine, although even these populations were adversely affected by the millimolar concentrations (data not shown) achieved with intrathecal administration.
In contrast with effects on Olig2+/BrdU+ populations in the CC, our analyses raise the possibility of a somewhat enhanced loss of DCX+ cells from among the BrdU+ population in both the SVZ and DG (Figure 12). In the SVZ, at 1 day after treatment, there was a disproportionate and significant reduction in the percentage of DCX+/BrdU+ cells, which represented 50 ± 3% of the cells incorporating BrdU in control animals and only 28 ± 8% in animals treated three times with cytarabine. This disproportionate reduction in the percentage of BrdU+ cells that was DCX+ did not seem, however, to be maintained over time in the SVZ, and at day 56 the proportion of BrdU+ cells that were DCX+ was not different in controls versus treated animals. In contrast, in the DG, a reduction in representation of DCX+ cells was also seen, except that in this case there was a marked 60% reduction in the proportion of BrdU+ cells that were DCX+ when day 56 results were compared with either controls of the same age or the proportionate representation of this population at day 1 after injury.
In the SVZ and the DG, cytarabine application was also associated with an increased representation of GFAP+ cells among the BrdU-incorporating populations. This increased representation of GFAP+ cells was seen at both day 1 and day 56 in the SVZ and on day 56 in the DG. In addition, BrdU+ cells that did not label with any of the cell-type-specific antibodies used in these studies were more prominent in treated animals than in controls at day 1 (but not at day 56) in the SVZ, and were found in the DG at both time points (data not shown). The only tissue in which these unlabeled cells provided a greater than 10% contribution to the entire BrdU+ population was in the DG. Such cells represented around 2% and around 20% of the BrdU-labeled cells at days 1 and 56, respectively, of all BrdU-labeled cells in control animals versus around 15% and about 35% (for days 1 and 56, respectively) of the entire BrdU+ population in the treated animals.
We found that normal neural progenitor cells and oligodendrocytes of the CNS are exceptionally vulnerable to the toxic effects of the chemotherapeutic agents BCNU, cisplatin, and cytarabine. Vulnerability to these drugs was observed for all classes of lineage-restricted progenitor cells that can be readily grown as purified cell populations. Moreover, vulnerability was not restricted to dividing cells, as nondividing oligodendrocytes were also targets of these drugs, at exposure levels routinely achieved during treatment. In vitro analyses of purified cell populations were highly predictive of effects seen following systemic treatment with any of the chemotherapeutic agents in vivo. Comparative analysis of multiple cancer cell lines from different tissues only identified one cell line in which vulnerability was comparable to that observed for primary neural progenitor cells, with most such cell lines being more resistant to these agents than the normal cells (despite often being chosen because of their previous use in studies on the response to the drugs studied). Thus, it appears that the vulnerability of multiple normal cell populations of the CNS to cisplatin, BCNU, and cytarabine rivals the vulnerability of cancer cells themselves. The fact that toxicities for neuronal precursors, glial precursors, and oligodendrocytes, and toxicity in three different regions of the CNS, are associated with systemic application of chemotherapeutic drugs is of particular concern, as such toxicity would be applicable to treatment of all forms of cancer. Moreover, our studies demonstrate that the adverse effects of systemic application are not limited to the classes of DNA cross-linking agents represented by BCNU and cisplatin, but also are observed with the antimetabolite cytarabine. Thus, the adverse effects observed in the present studies may be relevant in understanding the side effects of multiple classes of chemotherapeutic drugs.
This is the first study of which we are aware that demonstrates that neural progenitor cells and oligodendrocytes are exceptionally vulnerable to the action of chemotherapeutic drugs in vitro and in vivo, even when applied extra-cranially. This study also suggests that, at least in the CNS, it is progenitor cells and not stem cells that are the most vulnerable targets. Adverse effects are known to occur clinically with all the agents we studied, both acutely and as delayed neurotoxicities (such as cognitive impairment) that may only become apparent years after treatment. For example, BCNU treatment has been associated with significant changes in mental status and with white matter degeneration [23, 24]. Cisplatin at high doses has been associated with leukoencephalopathy and destruction of CNS white matter . Application of cytarabine, the third drug examined in our studies, has also been associated with acute encephalopathy, confusion, memory loss, and white matter changes [25, 62]. The vulnerability of neural progenitor cells and oligodendrocytes to these drugs, which was also observed in our antigenic analysis of TUNEL-labeled cells in the CNS of animals exposed to BCNU in vivo and BrdU-labeled cells exposed to either BCNU or cytarabine, may provide an explanation for the neurotoxic consequences of the treatments and also may be relevant to understanding long-term toxicities. It was particularly striking that O-A/OPCs and oligodendrocytes were one to two orders of magnitude more sensitive to cisplatin or cytarabine than has previously been observed in studies on multiple neuronal populations from both the CNS and the peripheral nervous system [65–70].
The toxicities seen in our studies occurred well within the concentration ranges achieved for these agents in CSF during cancer therapy. For example, cisplatin toxicity for multiple neural cell types was observed at concentrations as low as 0.1 mM (Figure 3). CSF concentrations for cisplatin in conventional or low-dose intravenous applications are between 0.6 and 2.8 μM  but can reach up to 80 μM in high-dose applications . Moreover, much higher concentrations in brain tissue and CSF have been reported after intra-arterial applications, liposomal encapsulations, after previous radiation, or in cases of blood-brain barrier disruption [37, 38]. BCNU toxicity was observed at concentrations as low as 5 μM. This agent is highly lipophilic, and about 80% of plasma levels are detectable in CSF and brain tissue . CSF concentrations of BCNU are in the range of 8–10 μM after intravenous applications , but can be 100–1,000-fold higher after local applications via biodegradable polymer wafers [39, 40]. Similarly, the toxicity of cytarabine was already apparent at concentrations as low as 0.1 μM or less, compared with CSF concentrations during conventional treatments in the range 0.1–0.3 μM, and concentrations that are ten times higher in high-dose applications, and 10,000 times higher following intrathecal application .
In vitro studies further indicated that the toxicity of BCNU, cisplatin, and cytarabine is not limited to the induction of cell death, but is also associated with the suppression of cell division of O-2A/OPCs even when applied transiently at levels that cause little or no cell death, and that represent small fractions of the CSF concentrations achieved with systemic chemotherapy. The suppression of division was particularly striking in that a single transient exposure of dividing O-2A/OPCs to BCNU, cisplatin, or cytarabine was sufficient to cause a marked reduction in subsequent cell division at the clonal level. Such a loss of dividing cells would compromise the ability of dividing progenitor cells to contribute to repair processes, and could also contribute to long-term or delayed toxicity reactions.
The observations that BCNU, cisplatin, and cytarabine all cause dividing O-2A/OPCs to undergo a greater extent of oligodendrocyte generation are as predicted from our studies on the role of intracellular redox state in controlling the balance between self-renewal and differentiation , and from observations that all three agents cause cells to become more oxidized [69, 71–75]. In our studies on redox regulation of precursor cell function, we found that O-2A/OPCs that are slightly (around 20%) more oxidized have a higher probability of undergoing differentiation, whether this oxidative status is due to cell-intrinsic mechanisms, exposure to pharmacological pro-oxidants or to physiological inducers of oligodendrocyte generation (such as thyroid hormone) [41, 43]. Even when this shift in differentiation probability is relatively small , cumulative effects over multiple cell generations can lead to differentiation outcomes in which clonal composition is clearly different but in which analysis at delayed time points is required for the reduction in progenitor cell representation to translate into markedly smaller clonal sizes.
In vitro studies on purified cell populations appeared to accurately predict sensitivities observed in vivo. Combined analysis of TUNEL and antigen expression demonstrated death of both neuronal and glial precursors, as well as of oligodendrocytes. Combined analysis of BrdU labeling and antigen expression similarly revealed reductions in BrdU incorporation in neuronal precursors of the hippocampus and in glial precursor cells of the CC. The high level of correlation between in vitro and in vivo outcomes suggests that purified populations of the cell types studied can provide a means of rapidly analyzing other cancer therapies.
Although all chemotherapeutic drugs examined were associated with toxicity in vivo, there were important differences between them. BCNU was associated with particularly severe and prolonged cell death in vivo, while cell death induced by cisplatin was less severe and eventually returned to normal values. Cytarabine was associated with increased cell death for at least 14 days after treatment ended, with values tending towards or at base-line levels of TUNEL labeling at 56 days post-treatment. Whether the less severe effects of cisplatin in this regard were due to different drug characteristics in terms of blood-brain barrier permeability is not known (although, in this regard, it should be noted that cisplatin application in vivo may actually cause opening of this barrier ).
All three agents examined were associated, moreover, with continued reductions in cell division in one or more CNS regions after treatment ended, suggesting a long-lasting depletion of populations required for cell replenishment. Nonetheless, the fact that some BrdU-incorporating cells remained in all brain regions examined raises the question of whether treatments analogous to those used to enhance bone-marrow function after cancer treatment may be applicable some day to enhancing the function of the normal dividing cells of the CNS during or after cancer treatment, possibly even using the same cytokines that are used to enhance cell repopulation from the bone marrow [78–80].
The effects of cytarabine on the different cell populations that incorporated BrdU in vivo were particularly surprising in the context of previous observations that cytarabine exposure in vivo (delivered by infusion onto the cortex for 7 days) is associated with a repopulation of the SVZ after treatment ceases [21, 81]. In contrast, our own studies indicate that this repopulation of dividing cells does not occur in the CC or DG, and may not endure in the SVZ (Figure 11). Although previous studies differ from our own in delivery methods and dosages applied, it may also be that the capacity for repopulation of dividing cells differs in different regions of the CNS. Moreover, it may be that the repopulation of the dividing cells of the SVZ is a transient phenomenon, as the latest time point examined in our studies was associated with a fall in the levels of BrdU incorporation to levels seen 1 day after treatment ended.
Taken together with recent studies on the effects of irradiation on the CNS , our results indicate that damage to CNS progenitor cells is an apparent correlate of both the main treatments for cancer. Monje et al.  suggested that the adverse effects of irradiation on the hippocampus might be causally related to the neurological symptoms and cognitive decline associated with this treatment. This suggestion would also apply to the effects of chemotherapy.
There are many ways in which the effects of chemotherapy may be even more of a concern than the effects of irradiation, beginning with the fact that whereas radiation damage is caused by therapy targeted to the CNS, toxicity after chemotherapy also occurs after systemic administration of these compounds. Moreover, our studies also reveal that the range of CNS cell types vulnerable to the effects of chemotherapy is greater than has been studied for irradiation, and demonstrate toxicity of chemotherapeutic agents for glial progenitor cells and for oligodendrocytes, as well as for the hippocampal precursor cells that have been examined in studies on the effects of irradiation . Yet another difference between the effects of these two modes of treatment is that irradiation-associated impairment of neurogenesis appears to be a secondary effect of inflammation, and can thus be reduced with anti-inflammatory agents . In contrast, our preliminary analyses of chemotherapy-treated animals have not revealed any increased microglial activation, a hallmark of CNS inflammation (J. D. and M. N., unpublished work). Thus, there is presently no reason to think the adverse effects of chemotherapy might be ameliorated by control of inflammation. The two sets of studies also differed in severity of outcome, in that our study reveals a partial fall in the representation of DCX+ neuronal precursor cells whereas the studies on irradiation revealed a virtually complete lack of neurogenesis . While it will be of interest to extend examination of both treatment paradigms, it is nonetheless the case that both studies raise the concern that neurogenesis in the brain is vulnerable to both forms of cancer treatment.
Our studies have multiple implications for future strategies of cancer treatment. As doses of BCNU, cisplatin, and cytarabine that killed even chemosensitive cancer cell lines were equally or more toxic for neural progenitor cells and oligodendrocytes, it seems that any concentration of these chemotherapeutic agents sufficient to harm cancer cells may also damage many cell populations of the CNS. That cisplatin may have less severe long-term effects than BCNU might be construed as encouragement that less toxic treatments can be developed with existing chemotherapeutic agents. It is also possible, however, that our results actually understate the extent of damage that occurs in association with chemotherapy. Such treatment is typically applied for several courses over an extended period of time. Furthermore, current treatment protocols simultaneously apply multiple different chemotherapeutic agents. This issue is of particular concern in the light of reports that agents such as cisplatin or BCNU can cause opening of the blood-brain barrier [77, 84], which could allow entry of adjunctive non-lipophilic agents into the CNS. In addition, there are multiple therapeutic regimes associated with higher concentrations of drugs than those we have studied (for example, intra-arterial administration, liposome-encapsulated drugs, or locally applied biodegradable wafers in the treatment of brain tumors). Moreover, the advances that have been made in rescuing patients from the toxicity of chemotherapeutic agents for bone marrow have been associated with a tendency to apply yet higher doses of these agents, thus potentially increasing the risk of neurotoxicity.
As chemotherapy will remain a cornerstone of cancer therapy for the foreseeable future, the potential ramifications of this work for present and future cancer treatments seem clear. Plainly, it is of great importance to identify the neural populations at risk during any cancer treatment in order to develop means of reducing neurotoxicity and preserving the quality of life in long-term survivors. This is an issue of great concern, particularly in the light of recent studies favoring the use of more aggressive and high-dose regimens or of newer drugs that target receptor tyrosine kinase signaling pathways that are critical regulators of neural progenitor and stem-cell function. In this context, it will be of particular importance to include more profound analysis of CNS toxicity in the assessment of new candidate chemotherapeutic drugs, an evaluation that currently is not consistently performed. It will also be critical to understand why some patients have adverse side effects (whether neurological or non-neurological), whereas others are spared such damage, and to determine the value of low-dose (metronomic) therapies  in avoiding damage to the CNS without compromising treatment outcome. In this regard, it is of concern that our in vitro results raise the possibility that even exposure to very low levels of these agents may compromise progenitor cell division. It is clearly vital to identify therapeutic approaches that do not share these problems, either by enabling targeted killing of cancer cells or through selective protection of normal cells during cancer treatment. The strong correlations between our in vitro and in vivo analyses indicate that the same approaches we used to identify the reported toxicities can also provide rapid in vitro screens for analyzing new therapies and discovering means of achieving selective protection or targeted killing. In light of the ease of use of these in vitro and in vivo assays, applying them early in the drug-discovery process may enable a more rapid identification of treatments able to eliminate cancer cells without compromising the patient's quality of life.
In vitro studies were performed on purified cultures of primary CNS cells. Multipotent neuroepithelial cell cultures were prepared from embryonic day 10.5 (E10.5) Sprague-Dawley rat spinal cord, as previously described [29, 86]. NRP cells were prepared by inducing neuronal differentiation from multipotent NEP cells, as described . Glial-restricted precursor cells (A2B5+ GRP) were isolated directly from E13.5 Sprague-Dawley rat spinal cord . Purified O-2A/OPCs were prepared from the CC or optic nerve of 7-day-old Sprague-Dawley rats using a specific antibody capture assay . Purified oligodendrocytes were generated from O-2A/OPC cell cultures by growing cells in presence of thyroid hormone (45 μM) to induce oligodendrocyte differentiation . Purified cortical astrocytes were prepared from 1- to 2-day-old Sprague-Dawley rats as described . Multipotent and lineage committed human embryonic neural progenitor cells were obtained from Clonetics (San Diego, CA, USA) and propagated as described previously [32, 88].
Brain tumor cells used in this study were isolated from patients with glioblastoma multiforme (1789, UT-12, UT-4 and T98 cell lines). Brain tumor cells were grown in serum-free conditions in 50% chemically defined medium (DMEM/F-12, supplemented with PDGF-AA and basic fibroblast growth factor (FGF) at 10 ng/ml each) and 50% astrocyte-conditioned medium (derived from cortical astrocyte cultures ). In addition, SW480 and HT-29 colon carcinoma cells, uterine (MES), breast (MCF-7 and MDA-MB-231), and ovarian cancer (ES-2) cells, L1210 lymphocytic leukemia and EL-4 lymphoma cells and a meningioma cell line, derived from a patient with a meningotheliomatous meningioma, were also evaluated. These cells were propagated in DMEM/F-12 in presence of 5% FCS, except for EL4 and L1210 (DMEM + 10% horse serum) and ES-2 (McCoy's 5A (Cellgro) + 10% FCS). Sensitivity of cancer cells to chemotherapeutic agents showed no significant differences whether cells were assayed in the presence or absence of serum.
For in vitro toxicity studies, cells were plated on coverslips at a density of 1,000 cells per well. After 24–48 h, cells were exposed to increasing drug concentrations of BCNU (5–200 μM) for 1 h, cisplatin (0.1–100 μM) for 20 h or cytarabine (0.01 μM to 2 μM) for 24 h. Cells were then allowed to recover for 24–48 h, the times being based on clinically applied dosages and elimination half-times of these drugs in vivo. Cell survival and viability was determined using the 3,(4,5-dimethylthiazol-2-yl) 2,5-diphenyl-tetrazolium-bromide (MTT) assay in combination with 4',6-diamidino-2-phenylindole (DAPI) staining to visualize DNA. The MTT assay was performed as described and also combined with immunofluorescence . This assay is more sensitive than the plate reader assay used in our previous studies on the effects of BCNU on oligodendrocytes, O-2A/OPCs, and astrocytes . After MTT and DAPI staining, surviving cells were determined by microscopically counting all individual cells in control and treatment groups. All counting was done blinded by a separate investigator. Each experiment was carried out in quadruplicate and was repeated at least twice in independent experiments. Data points represent mean from single experiments and error bars shown in figures represent ± standard error of the mean (SEM).
Cell cultures were immunostained as described [29–32, 41], using the following antibodies: A2B5 mouse IgM mono-clonal antibody (mAb) (Developmental Hybridoma Bank, Iowa City, IA, USA); anti-galactocerebroside mouse IgG3 (GalC, 1:1, Developmental Hybridoma Bank, 1:50); anti-GFAP polyclonal rabbit Ig (DAKO, Copenhagen, Denmark, 1:400); anti-neurofilament protein mouse mAb IgG1 (NF-L, Chemicon, Temecula, CA, USA, 1:200), and anti-b-III-tubulin mouse mAb IgG2b (Biogenex, San Ramon, CA, 1:400). Antibody binding was detected with appropriate fluorescent dye-conjugated secondary antibodies (10 mg/ml, Southern Biotechnology), or Alexa fluorophore-coupled antibodies at a concentration of 1 μg/ml (Molecular Probes, Eugene, OR, USA).
For in vivo experiments, CBA mice at 6–8 weeks of age were treated with chemotherapy under approved protocols. BCNU, cisplatin, or cytarabine were administered via i.p. injections. Animals received BCNU, cisplatin, or cytarabine as three consecutive injections (3 × 10 mg/kg, 5 mg/kg, or 250 mg/kg body weight, respectively). Control animals received equal amounts of 0.9% NaCl i.p. Animals were sacrificed on days 1, 10, and 42 after completion of treatment for cisplatin and BCNU (where day 0 equals the time of the very last injection of the agent). For all in vivo experiments, animals were perfused transcardially with 4% paraformaldehyde in phosphate buffer (pH 7.4), under deep anesthesia using Avertin (tribromoethanol; Sigma, St Louis, MO, USA; 250 mg/kg, 1.2% solution).
Free-floating sections (40 μm) were used for all in vivo experiments for TUNEL staining and combined immunofluorescence staining. Detection of nuclear profiles with DNA fragmentation, one of the hallmarks of apoptosis, was performed using a TUNEL assay on free-floating brain sections based on the ApopTag-In-Situ Cell-Death-Detection Kit (Intergene, Purchase, NY, USA), according to the manufacturer's recommendations. The TUNEL assay was followed by DAPI counterstaining to visualize nuclear profiles in all in vitro assays and when sections were analyzed in a fluorescence microscope.
Briefly, sections were rinsed in TBS (0.9% NaCl and 0.1 M Tris-HCl pH 7.5) for 10 min, then exposed to a series of increasing concentrations of ethanol (50%, 70%, and 90% for 2 min each), followed by a 10 min incubation in 100% ethanol and a decreasing series of ethanol in 90%, 70%, and 50% for 1 min each, followed by rinsing in distilled water. After three rinses in TBS, the sections were exposed to equilibration buffer for 1 min at room temperature, and reaction buffer (TdT solution) for 1 h at 37°C, as per the manufacturer's recommendations. The reaction was terminated using the Stop buffer for 10 min at room temperature. Sections were rinsed 3× in TBS and 1× in TBS+ (TBS/0.1% Triton X-100/3% donkey serum) for 1 h to reduce background staining. Fragmented DNA was detected by incubation of sections in an anti-digoxigenin-FITC (fluorescein isothiocyanate) antibody for 1 h at 4°C.
To combine TUNEL staining with immunofluorescence staining for different cell-lineage markers, TUNEL staining was carried out first, followed by exposure with either one of the following primary antibodies for 24 to 48 h: mouse anti-NeuN (1:500, Chemicon), mouse anti-DXC (double-cortin) (1:500, Santa Cruz, Santa Cruz, CA, USA), rabbit anti-active caspase-3 (1:1000, R&D systems, Minneapolis, MN, USA), rat anti-S-100b (1:2500, Swant, Bellinzona, Switzerland), rabbit anti-NG2 (1:2000, gift of William Stallcup, Burnham Institute, La Jolla, CA, USA), mouse anti-MBP (1:1000, Chemicon), mouse anti-CNPase (1:2000, Sigma) and rabbit anti-GFAP (1:2500, DAKO). All secondary antibodies, generated in donkey (anti-rat, anti-rabbit, and anti-mouse), were coupled to TritC, FitC or Cy5 (Jackson Immuno Research, West Grove, PA, USA) for in vivo staining and were used according to the species of primary antibody. Free-floating sections were incubated with secondary antibodies for 4 h in TBS+. All secondary antibodies were used at a concentration of 1:500. After several washes in TBS, sections were mounted on gelatin-coated glass slides using Prolong Antifade mounting medium (Molecular Probes).
Fluorescent signals were detected using a confocal laser-scanning microscope Leica TCS SP2 (Heidelberg, Germany) and a 40× oil-immersion lens. All fluorescent images were generated using sequential laser scanning with only the corresponding single wavelength laser line (488 nm, 568 nm, and 647 nm, for each fluorescent channel, respectively), activated using acousto-optical tunable filters to avoid cross-detection of either one of the fluorescence channels. In addition, pinhole settings corresponding to an optical thickness of less than 2 mm were used to avoid false-positive signals from adjacent cells.
To label the proportion of dividing cells engaged in DNA synthesis in vivo, mice received a single injection of 5-bromodeoxyuridine (50 mg/kg body weight), dissolved in 0.9% NaCl, filtered at 0.2μm, and applied i.p. 4 h before perfusion. Free-floating sections were treated with 0.6% H2O2 in TBS (0.9% NaCl and 0.1 M Tris-HCl pH 7.5) for 30 min to block endogenous peroxidase. For DNA denaturation, sections were incubated for 2 h in 50% formamide/2× SSC (0.3 M NaCl and 0.03 M sodium citrate) at 65°C, rinsed for 5 min in 2× SSC, incubated for 30 min in 2 N HCl at 37°C, and rinsed for 10 min in 0.1 M boric acid pH 8.5. Several rinses in TBS were followed by incubation in TBS/0.1% Triton X-100/3% donkey serum (TBS+) for 30 min and incubation with rat anti-BrdU antibody (Harlan Sera Lab, Loughborough, UK, 1:2500) in TBS+ overnight at 4°C. Sections were rinsed in TBS+ and incubated for 1 h with biotinylated donkey anti-rat antibody. Sections were rinsed several times in TBS and avidin-biotin-peroxidase complex (ABC system, Vector Laboratories, Burlingame, CA, USA) was applied for 1 h, followed by peroxidase detection for 5 min (0.25 mg/ml DAB, 0.01% H2O2, 0.04% NaCl). After several washes in TBS, sections were mounted on gelatin-coated glass slides using Prolong Antifade mounting medium (Molecular Probes).
To analyze BrdU incorporation in specific cell types, anti-BrdU immunostaining was combined with immunolabeling to identify DCX+ neuronal precursor cells, Olig2+ oligodendrocyte precursor cells (defined as cells that were BrdU+ and Olig2+, in order to discriminate these cells from Olig2+ nondividing oligodendrocytes [59–61]), and GFAP+ cells (which would have been astrocytes in the CC or DG or, in the SVZ, may also have been stem cells). Labeling and confocal analysis was carried out as for the combination of immunolabeling with TUNEL staining. A minimum of 50 BrdU+ cells were counted for each labeling condition in each animal (n = 3 animals in each group examined), with the sole exception of the DG of the animals examined 56 days after cytarabine treatment (for which an identical number of sections were examined as in control animals, but the frequency of labeled cells was not sufficient to reveal 50 cells in these sections). Rabbit anti-Olig2 antibody was a kind gift from David Rowitch.
Brains were cut coronally as 40-μm sections with a sliding microtome (Leica, SM/2000R) and stored at -20°C in a cryoprotectant solution (glycerol, ethylene glycol, and 0.1 M phosphate buffer pH 7.4, 3:3:4 by volume). Quantification of BrdU+ cells was accomplished with unbiased counting methods. BrdU-immunoreactive nuclei were counted in one focal plane to avoid oversampling. Brain structures were sampled either by selecting predetermined areas on each section (lateral subventricular zone = SVZ) or by analyzing the entire structure on each section (CC, DG of the hippocampus). Differences were considered significant when p < 0.01. SVZ: BrdU+ cells were counted in every sixth section (40 μm) from a coronal series between interaural anterior-posterior (AP) +5.2 mm and AP +3.9 mm (the anterior commissure crossing). BrdU+ cells were counted along the lateral ventricular wall up to 200 mm from the lateral ventricle wall. Corpus callosum (CC): BrdU+ cells were counted in every sixth section (40 μm) from a coronal series between interaural AP +5.2 mm and AP +3.0 mm in the entire extension of the rostral and medial part of the CC and analyzed as for SVZ. Dentate gyrus (DG) of hippocampus: BrdU+ cells were counted in every sixth section (40 μm) from a coronal series between interaural AP +2.5 mm and AP +1.1 mm. BrdU+ cells were counted in the area of the DG, including the hilus, subgranular zone (SGZ), and the granule cell layer (GCL) and analyzed as for SVZ. Quantitative data in all figures is presented as mean percentage normalized to control animals. Error bars represent ± SEM.
Digital images were captured using a Nikon Eclipse E400 upright microscope with a spot camera (Diagnostic Instruments, Sterling Heights, MI, USA) and the spot advanced software for Macintosh (Diagnostic Instruments), or using the confocal laser-scanning microscope (Leica TCS SP2). Photomicrographs were processed on a Macintosh G4 and assembled with Adobe Photoshop 7.0 (Adobe Systems, Mountainview, CA, USA). In all comparisons, unpaired, two-tailed Student's t-tests were used.
It is a pleasure to acknowledge helpful discussions with our colleagues regarding this research, and in particular discussions with Chris Proschel and Hartmut Land. This work was supported by NIH grant NS44701 (MN) and a generous fellowship from the James P. Wilmot Foundation (JD).
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