- Methodology article
- Open Access
High-throughput and single-cell imaging of NF-κB oscillations using monoclonal cell lines
© Bartfeld et al; licensee BioMed Central Ltd. 2010
- Received: 22 December 2009
- Accepted: 16 March 2010
- Published: 16 March 2010
The nuclear factor-κB (NF-κB) family of transcription factors plays a role in a wide range of cellular processes including the immune response and cellular growth. In addition, deregulation of the NF-κB system has been associated with a number of disease states, including cancer. Therefore, insight into the regulation of NF-κB activation has crucial medical relevance, holding promise for novel drug target discovery. Transcription of NF-κB-induced genes is regulated by differential dynamics of single NF-κB subunits, but only a few methods are currently being applied to study dynamics. In particular, while oscillations of NF-κB activation have been observed in response to the cytokine tumor necrosis factor α (TNFα), little is known about the occurrence of oscillations in response to bacterial infections.
To quantitatively assess NF-κB dynamics we generated human and murine monoclonal cell lines that stably express the NF-κB subunit p65 fused to GFP. Furthermore, a high-throughput assay based on automated microscopy coupled to image analysis to quantify p65-nuclear translocation was established. Using this assay, we demonstrate a stimulus- and cell line-specific temporal control of p65 translocation, revealing, for the first time, oscillations of p65 translocation in response to bacterial infection. Oscillations were detected at the single-cell level using real-time microscopy as well as at the population level using high-throughput image analysis. In addition, mathematical modeling of NF-κB dynamics during bacterial infections predicted masking of oscillations on the population level in asynchronous activations, which was experimentally confirmed.
Taken together, this simple and cost effective assay constitutes an integrated approach to infer the dynamics of NF-κB kinetics in single cells and cell populations. Using a single system, novel factors modulating NF-κB can be identified and analyzed, providing new possibilities for a wide range of applications from therapeutic discovery and understanding of disease to host-pathogen interactions.
- Automate Microscopy
- Mouse Fibroblast Cell Line
- Virus Integration Site
- Monoclonal Cell Line
NF-κB is a family of transcription factors that plays a critical role in regulating genes involved in cell proliferation, apoptosis, innate immunity, and inflammatory responses. NF-κB is activated by a range of physical and chemical signals including cytokines and bacterial (e.g. lipopolysaccharide; LPS) and viral products [1, 2]. Deregulation of the NF-κB system is implicated in many diseases including cancer [[3, 4], http://www.nf-kb.org]. Understanding the specificity and the temporal nature of NF-κB responsive gene expression is therefore not only of physiological interest but of crucial clinical importance.
Functional NF-κB is assembled through homo- or heterodimerization of the five subunits: p65 (RelA), RelB, c-Rel, p105/p50 (nfkb1) and p100/p52 (nfkb2). The classical dimer p65:p50 is ubiquitously expressed and is the primary mediator of inflammation . NF-κB dimers reside in the cytoplasm sequestered by inhibitor proteins, e.g. IκBα (Inhibitor of κBα), until a signal cascade is activated that leads to phosphorylation, ubiquitinylation and subsequent degradation of the inhibitor. As a result, the dimer translocates into the nucleus where it binds to DNA and triggers transcription of target genes. One of the target genes is the inhibitor itself creating a negative feedback loop. If the stimulus remains, repeated inhibitor degradation and re-synthesis can lead to oscillations of nuclear translocations. Further regulation mechanisms dampen the oscillations and finally lead to termination of the signaling cascade [2, 5–7].
Oscillations of NF-κB subunit nuclear translocation have been observed in single cells using fluorescence live-cell imaging [8–11]. Additionally, similar repeated cycles of DNA binding activity have been shown using the electrophoretic mobility shift assay (EMSA) in a range of cell types [12, 13]. In cell populations oscillations can be asynchronous due to phase interval heterogeneity in single cells [8, 9]. Dynamics of nuclear translocation or DNA binding can vary in response to different stimuli: While a sustained TNFα stimulus induces oscillations, a short pulse of TNFα leads to a single peak of activation ; LPS elicits, via secretion of TNFα and the subsequent overlap of the two signaling pathways (LPS and TNFα), a very heterogeneous response, with some cells displaying only one cycle of nuclear translocation, while other cells display oscillations or persistent nuclear translocation [11, 15, 16]. These observations have raised the possibility that NF-κB activation dynamics could determine gene activation specificity. Indeed, different frequencies of stimulation with TNFα induce different gene expression patterns [9, 12].
While oscillations have been shown in response to TNFα [8–15, 17, 18], the topoisomerase II inhibitor etoposide  and LPS  they have not yet been investigated during infection with live bacteria. The observation that oscillations occur in response to bacteria - being single units that naturally occur in infections - would be an important indication that they are physiologically relevant processes.
Although there are several methods to measure NF-κB activation, only some are suitable for investigating the dynamics of this signaling system. Commonly used tools for general NF-κB analysis are reporter plasmids, in which an NF-κB binding site drives the transcription of reporter genes like enhanced green fluorescent protein (EGFP) or luciferase. Stable cell lines with these constructs are commercially available (i.e. from Invitrogen) and similar constructs have been successfully used in analysis of other oscillators such as the circadian clock . However, these constructs and cell lines measure transcriptional responses accumulated after activation and therefore do not necessarily reflect the immediate translocation of NF-κB subunits to the nucleus in real time. In addition, many reporter constructs respond to several NF-κB dimers and do not report the activity of one particular NF-κB dimer.
Biochemical approaches like EMSA have been used successfully to detect oscillations in the temporal response of NF-κB [12, 15, 16, 18]. These experimental observations have also been simulated in a multivariable mathematical model of NF-κB activation dynamics . Although useful, biochemical approaches are time consuming and the protein extracts used for analysis average the potentially asynchronous responses of single cells.
Since activation of NF-κB is marked by the translocation of NF-κB subunits from the cytoplasm to the nucleus, many groups have used high-content image analysis of fixed and immunostained cells [20–22]. Other studies have followed the dynamics of NF-κB activation in live cells using fluorescent protein fusions [8–11, 14, 23–26]. Using the latter technique, Nelson and co-workers were the first to show NF-κB oscillations at a single-cell level [8, 9].
Here, we combined high-content automated fluorescence imaging of NF-κB protein subunit fusions with the stability of monoclonal cell lines to analyze the real-time dynamics of NF-κB activation within single cells. We have generated lentivirally transduced monoclonal cell lines expressing p65 fused to GFP that can be used in any microscopic analysis including high-throughput automated microscopy and live-cell imaging. Using these cell lines, we show inducer-specific temporal control of p65-translocations and, for the first time, oscillations in response to infection with the bacterium H. pylori. These experimental data were also used to construct a simplified mathematical model of NF-κB signaling regulation.
A high-throughput assay for monoclonal cell lines expressing p65-GFP
Comparison of parental and p65-GFP cell lines
Mathematical models have predicted that ectopic expression of NF-κB subunits could alter the dynamics of the signaling module , while experimental data have shown that this is not necessarily the case . Therefore, we compared NF-κB activation in parental, non-transduced cell lines with p65-GFP expressing cell lines. Western blot analysis showed both cell lines exhibited very similar patterns of IκBα degradation over a period of 90 minutes after stimulation with TNFα at 10 ng/ml or 0.5 ng/ml (Additional file 5a). However, while the overall degradation pattern is comparable, the p65-GFP expressing cell lines seem to be slightly faster in restoring IκBα to baseline levels (i.e. non-stimulated sample levels). Therefore, we do not completely exclude the possibility that expression of the p65-GFP fusion slightly alters signaling dynamics. The degradation of IκBα in parental and p65-GFP expressing cell lines corresponded well to the percentages of cells with nuclear p65 calculated using the automated p65-translocation assay (Additional file 5b).
Stimulus-specific temporal control of p65-GFP translocations
The resulting profiles were highly specific regarding cell lines and inducers (see Figure 3). The main characteristics were: (i) The ability to recognize a stimulus depended on the cell line. None of the human epithelial cell lines tested responded to LPS, whereas the mouse fibroblasts were unresponsive to H. pylori, suggesting strict stimulus specificity, probably due to differences in functional receptors or signaling pathways present in the respective cells. (ii) Temporal profiles were stimulus specific. A549 exhibited damped oscillations after infection with H. pylori, but stable translocation after stimulation with TNFα or IL-1β. Stable translocations in response to TNFα were verified by live-cell imaging of A549 cells (data not shown). (iii) The percentage of activated cells, but not the temporal profile, was variable to the dose of the inducer. A reduction in the dose of IL-1β in AGS or TNFα in L929 led to a reduction in percentage of activated cells. (iv) Thresholds were cell-line specific. Low-dose challenge of AGS with IL-1β produced low percentages of activated cells, while the same doses yielded a full response in A549 and L929 cell lines. (v) The duration of the response varied between cell lines. A549 generally showed much longer responses, implying more amplification of the signal or fewer dampening mechanisms in this cell line. (vi) Only minimal background p65-translocation activity was observed in all cell lines (i.e. no stimulus, time 0).
Bacterial infection induces oscillations of p65-GFP
We observed damped oscillations of p65 translocation in response to H. pylori using the high-throughput assay (Figure 3). This bacterium is equipped with a type four secretion system (TFSS) capable of injecting its cytotoxicity associated protein A (CagA) as well as bacterial peptidoglycan into its infected host cell. Consistent with previous studies that employed a variety of techniques to analyze H. pylori- induced NF-κB activity [29–32], the oscillations shown here were dependent on a functional TFSS but not on CagA or other factors possibly secreted into the medium by bacteria or cells (Additional file 6).
Modeling oscillations after bacterial infection
Here we describe a simple and cost-effective method amenable to high-throughput applications that combines the use of p65-GFP expressing monoclonal cell lines with automated microscopy and analysis to provide synchronous real-time analysis of NF-κB activation dynamics at a single-cell and population level. By applying this system, we reveal a single bacterium is apparently sufficient to induce translocation of p65-GFP. Moreover, we show single cellular variabilities in NF-κB dynamics, indicating the interplay of multiple parameters in the regulation of NF-κB.
There are many different oscillatory systems  and expression of fluorescent fusion proteins has been a useful tool to study dynamics of these oscillatory, and also non-oscillatory, signaling systems [8–11, 34–38]. Oscillations in NF-κB signaling have previously been shown using a variety of techniques and cell types [9–16]. To analyze oscillations on a single-cell level, most previous studies have relied on transient protein expression [8, 9] and discrepancies in oscillation synchrony between population and single-cell analysis has been discussed to result from different expression levels of the fusion protein in single cells ; however, experimental data has shown this is not necessarily the case . Most importantly, NF-κB oscillations and heterogeneity in peak intervals are comparable between different studies using transient expressions [8, 9], clonal cell lines (in which all cells have the same expression level) [9, 11], stable expression on the endogenous level  or a GFP-p65 knock-in mouse model with endogenous p65 levels . Moreover, the reported oscillations match the moderate asynchrony observed here (see Figure 4).
Advantages of the assay systems presented here are the lentiviral transduction of the p65-GFP expressing gene and its stable integration into the cellular genome. This not only avoids continued selection pressure for maintaining gene expression but allows the establishment of well-defined cell lines. Virus integration into the host cell genome is statistically unlikely to disrupt any relevant gene functions; however, this can be ascertained by sequencing the integration sites. Consistently, a comparison with the parental cells showed little influence of ectopic expression at the level of IκBα degradation (Additional file 5). Moreover, the assay system requires no extra material, avoiding unnecessary addition of experimental variables and making it highly cost-effective. Lastly, the method exhibits high sensitivity as background activity levels are very low (Figure 3).
The p65-GFP carrying lentivirus itself also offers interesting features for future approaches: Not only can it be used to generate any other cell line desired but, as lentiviruses can even infect non-dividing cells, it can be applied to the transduction of primary cells. Notably, one can influence the expression level of p65-GFP by varying the copy number of viruses per cell, i.e. using higher virus titers would lead to high numbers of integrated copies per genome and thus to higher expression levels.
Here, we observed inducer- and cell line- specific signatures of NF-κB response patterns (see Figure 3). The p65-GFP protein exhibited either oscillating translocation or rather stable activation; the percentage of activated cells varied with the dose of the inducer. Both observations are generally consistent with previous findings [15, 16, 39]. Stimulus-specific temporal control of NF-κB activation has also been observed in mouse embryonic fibroblasts (MEFs) using EMSAs: when stimulated with TNFα they displayed oscillatory behaviour, but when stimulated with LPS they displayed stable behaviour. The stable activation could be attributed to a positive feedback that leads, via the secretion of TNFα, to an overlap of two signaling pathways, both oscillatory when isolated but leading to stable activation when overlapping [15, 16]. Live-cell analysis of single cells revealed that the stable activation observed on the population level was due to the highly heterogenous responses of single cells resulting from a noisy paracrine TNFα signal . Possibly a similar mechanism lays beneath the stable activation observed here after TNFα or IL-1β induction, but as TNFα leads to a single translocation in A549 with the stimulus remaining in the medium, it seems unlikely that a potential feedback loop in this case involves TNFα. The same applies to the stimulation with IL-1β.
NF-κB oscillations have been observed in cell culture models using relatively high doses of inducers such as TNFα [8–12, 14, 15, 17, 18] and LPS . Data presented here show, for the first time, oscillations in response to bacterial infection and that a single bacterium seems to be capable of inducing p65 translocation. Therefore, oscillations are likely to occur in infections in vivo. As with other inducers of NF-κB such as TNFα [8–11, 14], H. pylori infection elicited a moderate cell-to-cell variability in p65 oscillations (Figure 4). Future experiments will clarify whether the observed variations of peak intervals in single-cell oscillations are due to stochastic transcription of the IκBα gene, as suggested recently , or can be attributed to the strength of induction and/or repeated infection by individual bacteria, as likely found during bacterial infection in vivo.
Based on these experimental data, we developed a simple mathematical model of NF-κB signaling temporal regulation. While our model of the NF-κB cascade may appear somewhat simplifying and might have been formulated in a much more elaborate fashion [2, 12, 28], we were not aiming for a detailed representation of the mechanisms or potential mechanisms leading to oscillations. Rather our goal was, given the experimental fact of oscillations, to correlate single-cell observations and population events derived from two different experimental approaches . Mathematical modeling will be an important tool for linking observations on different levels of granularity and using different technologies . In our situation a more complicated model of the single cell probably would not improve our understanding of the collective observations. Integrating our observations that oscillations of single cells can be masked at a population level by asynchronous stimulations, each stimulation being a discrete event dependent on MOI, we demonstrated the unique ability of our cell model to indicate differential dynamics at the population and single-cell levels. Data generated using the clonal cell lines could be used to refine and broaden our and similar mathematical models by providing experimental details of population and single-cell level oscillations within different cell types.
Owing to the crucial roles that NF-κB plays in inflammation, immunity and cancer, both the pharmaceutical industry as well as research groups are actively pursuing the discovery of new compounds that modulate NF-κB . The cell lines and the high-throughput microscopic assay presented here could be of considerable value for these efforts, providing a highly cost-effective method to identify and further analyze promising novel factors using one system; for instance, an RNAi-based screen could identify factors that prolong or inhibit dampening of oscillations, thereby opening new avenues of therapeutic discovery and understanding of disease. Analysis of temporal profiles of NF-κB activation in infections can unravel sequential activations and even provide indications for the inducing stimulus . Furthermore, the combination of novel live-cell imaging technologies with mathematical modeling at the single-cell and cell-population level may lead to a better mechanistic understanding of the host-pathogen interaction governing infections.
Lentiviral vector construction and transformation
p65-GFP was a kind gift from Johannes A. Schmid  and was cloned into pWPXL (kindly provided by Didier Trono http://tronolab.epfl.ch/) using the primers 5'-AATAATCGACGCGTCGATGGTGAGCAAGGGCGA-3' and 5'-ACCACCCACTAGTGTTAGGAGCTGATCTGACTCAG-3'and MluI and SpeI sites. GFP used is the eGFP from Clontech. The resulting construct pSIB02 has been confirmed by sequencing. Lentiviral vector particles were generated by transient transfection of 293T using envelope and packaging vectors pMD2.G and psPAX2 (also kindly provided by Didier Trono). Virus particles were harvested from the supernatant 48 h post transfection and concentrated by ultracentrifugation at 25 000 rpm. AGS (ATCC CRL 1739, human gastric adenocarcinoma epithelial cell line), A549 (ATCC CCL-185, human lung carcinoma epithelial cell line) and L929 (ATCC CCL-1, mouse fibroblast cell line) were infected with lentiviral particles. Three days post infection, cells were singularized by serial dilutions, separation was confirmed by eye and monoclonal cell lines AGS SIB02, A549 SIB01 and L929 SIB01 were propagated.
Virus integration sites
DNA was isolated using DNeasy tissue kit (Qiagen) according to the manufacturer's instructions. For determination of the virus integration sites, the LTR region (which borders the integration site) of the integrated lentivirus was linearly amplified  using the forward primer LTR0-Biotin: 5'-agttaccagagtcacacaacagacg-3' (5' Biotin). Amplified DNA was purified using streptavidin-coated magnetic beads which bind the biotinylated LTR0 primer (Dynal magnetic beads; Invitrogen, according to the manufacturer's instructions). A second strand was synthesized using random hexamer primers (Roche), 2 U Klenow fragment (Roche) and 250 μM dNTP. To further amplify the LTR/genomic border, a second (nested) linear amplification was carried out using forward primers in the LTR of the integrated lentivirus (LTR1-Biotin: 5'-taagcagtgggttccctagttagc-3'). DNA was purified and digested as above and ligated to a double stranded MseI adapter (ABI), yielding a double stranded DNA fragment containing the LTR/genomic border with known ends. To further amplify these fragments, two sequential PCRs using forward primers in the LTR of the integrated virus (1st PCR using primer LTR1: 5'-taagcagtgggttccctagttagc-3', 2nd PCR using primer LTR3: 5'-cagagagctcccaggctcag-3'), and a reverse primer in the MseI adapter (5'-ggtcagatgagtcctgagtaa-3') were carried out. PCR products were separated on 3% agarose gels (Biozyme Sieve 3:1), extracted and purified using the Qiaquick Gel Extraction Kit (Qiagen), and then sequenced using primer LTR2: 5'-ccaggctcagatctggtctaac-3'. PCRs, capillary electrophoresis and sequencing were carried out by Services in Molecular Biology GmbH, Berlin.
Cell culture and bacterial culture
Cell lines were grown in RPMI (AGS and L929) or DMEM (A549) supplemented with 10% fetal calf serum (FCS), 2 mM L-glutamate and 1 mM NaPyruvate (DMEM only). H. pylori clinical isolate P1 and deletion mutants thereof were routinely cultured on horse serum agar plates under microairophilic conditions, as described previously .
Automated microscopy and image analysis
Cells were seeded in 96-well plates, one or two days prior to activation to obtain a confluency of approximately 70%. Before activation, medium was replaced by fresh medium (50 μl per well). For activation, another 50 μl of medium containing recombinant human TNFα (BD Pharmingen, 4-12 × 108 units/mg), recombinant IL-1β (Strathmann Biotech, 1 × 107 units/mg), LPS from Salmonella typhosa (Sigma), or H. pylori strain P1 at the appropriate concentration was added. After the respective incubation time, cells were fixed with 100% ice-cold methanol, stained with Hoechst 33342 (2 μg/ml) and stored in phosphate buffered saline (PBS) containing 0.1% NaN3. Four images per well were taken by the automated microscopy system Scan^R (Olympus) using autofocus on nuclei. Images were subsequently analyzed by Scan^R software (Olympus) and quantification of p65-translocation was carried out using a modified existing protocol . Here, nuclear areas were identified by Hoechst staining and around every nucleus a one-pixel-wide cytoplasmic area was set. To define compartments as accurately as possible, the nuclear area was eroded by two pixels and the cytoplasmic area was distanced by one pixel from the nucleus (see Figure 2). In the case of L929, the nuclear region was eroded by three pixels and the distance from the cytosol was two pixels. While the setting of subcellular regions was similar to an assay described previously for cells stained with anti-p65 antibodies , the analysis of p65-translocation was based on a different strategy. Here, we used software to depict cells in dot plots and set the regions as shown in Figure 2. Subsequently, gates were defined: cells in regions R01, R02 and R03 were defined as cells with mainly nuclear p65-GFP whereas cells in regions R01, R02 and R04 were defined as cells with mainly cytoplasmic p65-GFP. Numbers of cells with nuclear or cytoplasmic p65-GFP in every well were counted by the software. The percentage of cells with nuclear p65-GFP per well were calculated using Microsoft Excel (Percentage of cells with nuclear p65-GFP = cells with nuclear p65-GFP/sum of cells with nuclear and cytoplasmic p65-GFP × 100). Definition of regions and gating was optimized for every cell line and the same assay was used for every experiment. Graphs were compiled using Microsoft Excel or Sigma Plot 8.0.
Cells were grown in 3.5 cm2 glass bottom dishes (MatTek). Before infection, medium was changed to medium without phenolred (Invitrogen). Bacteria were harvested in the same medium, stained with Syto 61 (Molecular Probes) according to the manufacturer's recommendations and washed three times. The staining of bacteria fades after some minutes. Images were acquired every two minutes. Microscopy was carried out in a humidified incubator (37°C, 5% CO2) using the VT-Infinity system (Visitron Systems). The system is compiled of an Olympus IX81 (Olympus, Japan), VT-Infinity galvo scanner confocal head (Visitron Systems) and a Hamamatsu C9100-02 CCD camera (Hamamatsu Photonics K.K). Images were acquired and processed using MetaMorph (Universal Imaging Corporation) software.
Proteins from lysed cells were solubilized in Laemmli buffer, separated by SDS-PAGE, transferred to PVDF membranes, probed with p65 (Santy Cruz) primary antibodies and HRP-conjugated secondary antibodies (Amersham), and detected with ECL reagent (ICN). Signals were visualized on a phosphorimager (Phosphorimager, FLA-3000 Series; Fuji), and band intensities quantified by 1D evaluation using AIDA software (Raytest). Expression levels were calculated as the mean of five independent experiments.
We thank Jörg Angermann for outstanding technical assistance, Alexander Karlas and Hajar Habibi for help with lentiviral work, Hans Thorn and Anette Rejman Lipinski for assistance with live-cell microscopy, Didier Trono and Johannes A. Schmid for plasmids, Martin Meixner for determination of lentiviral integration sites and Stefan Moese for helpful discussions and ideas. This work was supported by funding under the Sixth Research Framework Programme of the European Union, Project INCA (LSHC-CT-2005-018704) and by the BMBF through the RNAi-Net (Grant No. 0313938A) to TFM.
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