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BioMed Research International
Volume 2014 (2014), Article ID 641647, 11 pages
Effects of Growth Phase and Temperature on Activity within a Listeria monocytogenes Population: Evidence for RsbV-Independent Activation of at Refrigeration Temperatures
1Bacterial Stress Response Group, Microbiology, School of Natural Sciences, National University of Ireland, Galway, Ireland
2Waters Corporation, Milford, MA 01757, USA
3Regenerative Medicine Institute (REMEDI), National Centre for Biomedical Engineering Science, National University of Ireland, University Road, Galway, Ireland
Received 4 October 2013; Accepted 5 December 2013; Published 5 March 2014
Academic Editor: S. L. Mowbray
Copyright © 2014 Marta Utratna et al. This is an open access article distributed under the Creative Commons Attribution License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original work is properly cited.
The alternative sigma factor of Listeria monocytogenes is responsible for regulating the transcription of many of the genes necessary for adaptation to both food-related stresses and to conditions found within the gastrointestinal tract of the host. The present study sought to investigate the influence of growth phase and temperature on the activation of within populations of L. monocytogenes EGD-e wild-type, ΔsigB, and ΔrsbV throughout growth at both 4°C and 37°C, using a reporter fusion that couples expression of EGFP to the strongly -dependent promoter of lmo2230. A similar activation pattern within the population was observed in wt-egfp at both temperatures, with the highest induction of occurring in the early exponential phase of growth when the fluorescent population rapidly increased, eventually reaching the maximum in early stationary phase. Interestingly, induction of activity was heterogeneous, with only a proportion of the cells in the wt-egfp population being fluorescent above the background autofluorescence level. Moreover, significant RsbV-independent activation of was observed during growth at 4°C. This result suggests that an alternative route to activation exists in the absence of RsbV, a finding that is not explained by the current model for regulation.
The ability of Listeria monocytogenes to cause foodborne listeriosis depends on a multifaceted stress response that is activated under conditions related to food processing including high concentrations of salt, acidic pH, limited oxygen, antimicrobial agents, and a wide range of temperatures from −0.4 to 45°C . The remarkable adaptability of this bacterium is partly modulated by transcriptional regulators that tailor gene expression to the conditions encountered, with a pivotal role being played by sigma factors that target RNA polymerase to specific promoter sequences . The alternative sigma factor, sigma B , first identified in L. monocytogenes based on homology to the general stress response sigma factor from the nonpathogenic bacterium Bacillus subtilis [3, 4] coordinates the response to a range of stresses as evidenced by the pleiotropic phenotypes associated with a sigB deletion (reviewed by ). A core set of -dependent genes ( regulon) has been described in L. monocytogenes and shown to be upregulated in response to a range of conditions including osmotic stress, cold shock, heat shock, acid stress, during stationary phase of growth, and under conditions encountered in gastrointestinal tract [3, 6–9]. There is significant overlap between the PrfA virulence regulon and the regulon  with evidence that may even modulate PrfA activity at the intracellular stage of infection . Thus plays important roles in both virulence and in the general response to stress, which makes understanding its regulation essential for future strategies that aimed at controlling this pathogen in the food chain and within the host.
The current model of activation in L. monocytogenes is based on the high level of similarity of the sigB operon to that from B. subtilis (rsbR-rsbS-rsbT-rsbU-rsbV-rsbW-sigB-rsbX) and it suggests posttranslational regulation of activity together with autoregulation at the transcriptional level . In the absence of stress stimuli interacts with an antisigma factor, RsbW, which renders it unavailable for interaction with RNA polymerase. The dephosphorylation of the anti-anti-sigma factor RsbV, which occurs in response to stress, is catalysed by the protein phosphatase RsbU. This renders RsbV capable of interacting with RsbW, which in turn liberates , allowing it to participate in transcription. RsbU activity is in turn regulated through an interaction with RsbT, whose availability is determined by its association with a high molecular weight (~2 MDa) stress sensing complex called a “stressosome”. B. subtilis environmental (physical and chemical) stresses influence activity in this way but energy-related stresses are transduced by an alternative phosphatase called RsbP. Since no homologue of RsbP is encoded in the genome of L. monocytogenes both environmental and energy stresses are proposed to be transmitted through RsbU [13, 14], but in both organisms the initial stress sensing mechanism remains to be elucidated.
Several studies have investigated the role of in allowing L. monocytogenes to grow at low temperatures. However studies addressing the effects of a sigB deletion on the phenotypic characteristics of L. monocytogenes at low temperature have reported conflicting observations. A ΔsigB strain of L. monocytogenes 10403S had reduced growth in a defined medium (DM) at 8°C  and L. monocytogenes EGD-e ΔsigB was reported to be sensitive to freeze-thaw cycles . In contrast, a ΔsigB derivative of L. monocytogenes EGD did not show impaired growth in DM at 3°C  and L. monocytogenes 10403S ΔsigB had a similar growth pattern to the wild-type when grown at 4°C in BHI over 12 days [17, 18]. The available evidence is also unclear on the question of whether of activity is elevated during growth at low temperatures. Transcription of the autoregulated sigB operon is induced at cold temperatures suggesting that activity is elevated during low temperature growth [3, 19]. The promoter of the opuC operon, which encodes a compatible solute uptake system known to be regulated by [20–22], has also been used to look at activity at low temperatures. One study reported that opuCA transcript levels are unaffected during temperature downshift or growth at 4°C , while another study observed that opuCA transcription is induced after temperature downshift . However, the presence of a -dependent promoter upstream from opuCA makes interpretation of these results more difficult . Thus the uncertainty in the literature regarding the role and regulation of during cold adaptation made it important to investigate this question further.
To clarify the role and activity of during adaptation to low temperature growth we have monitored activity during prolonged growth at 4°C in comparison to a culture growing at 37°C. activity was monitored by measuring the expression of two genes known to be under direct control, opuCA, and lmo2230, which encodes a putative arsenate reductase [20, 23]. Polyclonal antibodies were used to detect the OpuCA protein while lmo2230 expression was monitored using an EGFP (enhanced green fluorescent protein) reporter fusion to the strongly -dependent promoter of the lmo2230 gene [22, 24]. Fluorescence measurements were made using flow cytometry throughout growth in wild-type, ΔsigB and ΔrsbV backgrounds. The measurements revealed heterogeneous activation of within growing populations of cells, with increased activation evident as cells progressed through exponential phase, reaching maximum activation in stationary phase. Similar results were observed at both growth temperatures suggesting that activity was not increased by reduced temperatures per se. The study provides important new insights into the temporal and population-related parameters that modulate the activity of sigma B in L. monocytogenes.
2. Materials and Methods
2.1. Growth Conditions
L. monocytogenes EGD-e strains used in this study are listed in Table 1. For growth and flow cytometry (FCM) experiments at 37°C overnight cultures (16 h) were inoculated into 25 mL of sterile Brain Heart Infusion (BHI) broth (LabM) in 250 mL flasks to give a starting OD600 0.05. OD600 readings that were taken from rotary (180 rpm) shaken cultures at 45 min intervals over 7 hours and samples of cells were taken for FCM and fixed as previously described . Growth at 4°C was also monitored from a starting OD600 0.05. Stationary culture cells grown in BHI at 37°C were inoculated into 200 mL of sterile BHI in 2 L flasks and gently agitated (30 rpm) on the rocker (Stuart See-Saw Rocker SSL4) at 4°C. Samples were taken daily over 12 days for monitoring OD600 and at 3-day intervals for FCM.
2.2. Protein Extraction
For determining levels of bacterial cultures were grown in 50 mL of BHI for 3 h at 37°C. Then 1 mL of culture was transferred at 60 min intervals into a tube containing chloramphenicol at a final concentration of 10 μg mL−1 to prevent further protein translation during the sample preparation steps. Samples were stored on ice until the completion of the experiment. Each 1 mL culture was then centrifuged at 12,000 g for 10 min to pellet bacterial cells. The supernatant was discarded and each cell pellet was resuspended in 100 μL of BugBuster cell lysis reagent (Novagen, USA) containing 1% (v/v) DNaseI, 1% (v/v) Halt Protease Inhibitor Cocktail, and 1% (w/v) Lysozyme (Sigma, USA). Each cell suspension was then incubated at 37°C for 1 h with agitation. The resulting cell lysates were centrifuged at 5,000 g for 10 min to remove insoluble material. For OpuCA levels large-scale protein extraction was carried out by growing bacterial cultures at 37°C with a volume of 500 mL and removing 50 mL of cultures at 50 min intervals into a tube containing chloramphenicol at a final concentration of 10 μg mL−1. A disruption of cells was accomplished by sonication and protein extraction was performed as previously described . For EGFP and RsbW levels proteins were extracted from 100 mL of stationary cultures grown for 12 days at 4°C using the sonication-based method with a slight modification; cells were fixed in 1 : 1 volume of ice cold 1 : 1 (v/v) methanol/ethanol mixture for 10 min at −20°C before centrifugation. The concentrations of protein extracts were determined by the RC DC Protein Assay Kit (BioRad). The purified protein extracts were stored at −20°C until required.
2.3. Polyclonal Antisera Generation
DNA sequences corresponding to rsbW and sigB were PCR amplified from L. monocytogenes EGD-e using primers listed in Table 2. Each gene fragment was then cloned into pET101D with T7 promoter to include a 3′ polyhistidine tag for downstream purification requirements, yielding pEC02 and pEC03 which were transformed into E. coli BL21 (DE3). Cultures of E. coli harbouring either rsbW-his6 or sigB-his6 were grown in LB broth supplemented with 100 μg mL−1 ampicillin and induced for overexpression by addition of 1 mM IPTG at approximately OD600 of 0.5. Cells were grown for 4 h following induction and collected by centrifugation at 10,000 g, washed with sterile media, and lysed with Bugbuster (Novagen, USA) containing 0.1% (v/v) DNaseI. The bacterial cell lysate was partitioned between soluble and insoluble material by centrifugation at 10,000 g for 10 min. Recombinant proteins present as inclusion bodies were purified from the insoluble fraction by Ni-NTA affinity chromatography using buffers supplemented with 8 M urea. RsbW-His6 and SigB-His6 were subsequently purified and prepared as 2 mg mL−1 stocks for immunization carried out by Fusion Antibodies (Belfast). For each protein two NZW rabbits were injected at several sites on each animal with 1 mL of each recombinant protein stock solution supplemented with Freund’s adjuvant. 35 days following boosting serum from individual rabbits was tested for specificity against each target antigen. Approximately 5 months after-immunization antiserum against each antigen was collected. The rabbit anti-RsbW and anti-SigB IgG from each rabbit serum was isolated using protein A chromatography. Each IgG preparation was tested for specificity against target antigens using Western blotting.
2.4. Western Blotting
Western blotting analyses were performed using polyclonal antisera (1°Ab) developed in rabbits against and RsbW (this study) or in chickens against OpuCA  and against GFP (Abcam) with commercial secondary antibodies (2°Ab) HRP-conjugated anti-rabbit or anti-chicken (Promega) at appropriate dilutions (Table 3) in 3% w/v skim milk. Protein extracts were normalized to 5 mg mL−1 total protein concentrations and 10 μL of these samples was separated by SDS-PAGE and transferred to a nitrocellulose membrane. Membranes were blocked for 60 min in 3% (w/v) skim milk at room temperature and incubated overnight at 4°C with an appropriate 1°Ab. Incubations with 2°Ab were performed at room temperature for 60 min. Three ten-minute-long washing steps with Tween20 (Promega) diluted in PBS (Table 3) followed by 10 min in PBS were performed after each incubation with 1°Ab and 2°Ab. Blots were viewed with a chemiluminescent substrate (SuperSignal West Pico Chemiluminescent Kit, Pierce) using a light sensitive film (Amersham Hyperfilm ECL, GE Healthcare) or FluorChem Imager (Alpha Innotech Corp) and FluorChem IS-8900 software.
2.5. Flow Cytometry
FCM compared fluorescence of the fusion strains (wt-egfp, ΔsigB-egfp, ΔrsbV-egfp) to one another. The parent strains (wt, ΔsigB, ΔrsbV) were used to determine the level of autofluorescence and to define the EGFP gate above it. Analyses were performed with a BD Accuri C6 flow cytometer (Accuri Cytometers, Inc.) on 100 μL of the fixed and PBS-suspended cells from 96 round bottom plates (Sarstedt). The 488 nm blue laser excitation, FL1 533/30 nm (e.g. FITC/GFP) emission channel, and 66 μL/min flow rate were used. Each sample was performed in biological triplicate with duplicate analyses in each replication. A minimum of 100,000 events for each sample were recorded and processed with BD CFlow Software to determine % of fluorescent population and mean fluorescence values.
2.6. Visualization of the Fluorescence with Microscopy
One mL aliquots of bacterial cells was harvested with benchtop centrifuge at room temperature and subsequently resuspended in 50 μL of sterile PBS. Five μL of the suspension was smeared on microscope slides for visualization with Nikon Eclipse E600 microscope with a CCD camera attached using the B-2A filter and 1/8 Neutral Density (ND8) filter set. Images were recorded and processed for publication with ImageJ 1.44 software.
3.1. Activity Is Not Correlated with Cellular Levels of Protein
Stationary phase is known to induce -dependent gene expression [3, 25] and sigB itself is known to be autoregulated at the transcriptional level. To determine if the levels of changed during growth at 37°C Western blotting was performed on protein extracts taken at 60 min intervals from early exponential to stationary phase using anti- polyclonal antibodies. Surprisingly, the highest levels of were observed in the exponential phase of growth and levels decreased when the cells entered stationary phase (Figure 1(a)). However, the model for regulation established in B. subtilis suggests that activity in L. monocytogenes is modulated primarily at the posttranslational level by a partner switching mechanism . Thus availability of rather than levels determines its involvement in transcription. To determine when was active during growth in L. monocytogenes the expression of the -dependent gene opuCA was measured at protein level. OpuCA levels were shown to be significantly lower in exponential phase of growth than observed in stationary phase in L. monocytogenes EGD-e grown at 37°C (Figure 1(a)). Furthermore, OpuCA was not detectable in the ΔsigB background at any point of growth confirming -dependent expression of opuCA under the conditions tested. During growth at 4°C OpuCA levels were measured in exponential phase and compared to the corresponding extracts from 37°C growth. OpuCA levels were increased at 4°C in comparison to 37°C (Figure 1(b)). However, significant levels of OpuCA were detected in the ΔsigB background suggesting that opuCA is expressed, at least partly, in a -independent manner at 4°C, a finding that is consistent with an earlier transcriptomic study . Thus OpuCA levels are not a reliable indicator of activity during growth at refrigeration temperatures.
3.2. Is Activated during Exponential Growth at Both 37°C and 4°C
To develop an understanding of how the activity of changes during growth and to investigate an effect of cold temperature on activity, changes in lmo2230-promoter-driven fluorescence of egfp-tagged strains were analysed using flow cytometry at 4°C and at 37°C, at intervals of three days and 45 min, respectively (Figures 2(a) and 2(b)). As expected SGR values for fusion strains grown at 4°C were much lower than those recorded during growth at 37°C (Figure 2(c)).
Flow cytometry of wt-egfp cells grown at 4°C showed that the fluorescent population increased during the exponential phase of growth from 9.2% to 15.1% in days 3 and 6, respectively (Figure 3(a)). The highest proportion of fluorescent cells was observed in early stationary phase, reaching 36.6% of the population. The level of EGFP-expressing cells within late stationary phase cultures dropped to 24.7% suggesting that activity decreased slightly at 4°C during stationary phase. During growth at 37°C a very similar activation pattern was observed—in early exponential phase 11.2% of cells were found within EGFP-expressing gate while in mid-exponential phase 21.6% cells were recognised as fluorescent (Figure 3(b)). A further increase to 28.3% was observed in late exponential phase. During the stationary phase of growth at 37°C activity did not increase at the rate observed when cells were dividing and the population of fluorescent cells remained stable with values around 35%. Based on the proportion of fluorescent cells within the population, revealed using flow cytometry of wt-egfp strain, a similar activation pattern was observed both at 37°C and 4°C, with activity increasing in the early exponential phase of growth and reaching a maximum level in stationary phase.
3.3. An Alternative Route of Activation Exists at 4°C in the Absence of RsbV
To determine whether activity observed in wt-egfp strain (Figure 3) depends solely on and RsbV during growth, similar flow cytometry analyses were performed in ΔrsbV and ΔsigB backgrounds at 4°C and at 37°C at intervals of three days and 45 min, respectively (Figures 2(a) and 2(b); Supplementary material Figure , see Figure S1 in Supplementary Materials available on line at http://dx.doi.org/10.1155/2014/641647). All activity (i.e., EGFP-based fluorescence) was abolished in a ΔsigB background at both temperatures. Surprisingly, at 4°C cells of the ΔrsbV-egfp strain emitted fluorescence above the level of autofluorescence observed for the parent ΔrsbV strain (Figure 4(a)). In early exponential phase (day 3) 2.2% of population was recognised as EGFP-expressing while the proportion increased to 5.1% in late exponential phase (day 6). A further increase of the fluorescent population was observed in early stationary phase of growth where it reached its highest level of 19.8% (day 9) at 4°C. In late stationary phase (day 12) population of cells emitting fluorescence above autofluorescence background decreased to the level of 10.9%. In contrast to 4°C, none of the analysed populations of ΔrsbV-egfp or ΔsigB-egfp revealed significant fluorescence above the background at any stage of growth at 37°C (Supplementary material Figure ), suggesting that all EGFP expression observed with flow cytometry in wt-egfp population at 37°C was both - and RsbV-dependent.
To evaluate the finding of RsbV-independent expression of EGFP at 4°C microscopic observations of wt-egfp, ΔsigB-egfp and ΔrsbV-egfp cells were performed. Both the wt-egfp, and ΔrsbV-egfp cultures contained fluorescent cells at 4°C, whereas none of the fields captured for a ΔsigB-egfp culture had fluorescent cells (Figure 4(b)). To rule out the EGFP expression in ΔsigB background at 4°C (noncell-shaped fluorescent particles), proteins were extracted from 100 mL of the fusion strains cultures grown to stationary phase (day 12) (Figure 4(c)). EGFP was detected using Western blotting with anti-GFP antibody in protein extracts from the wt-egfp and low but detectable levels were observed in ΔrsbV-egfp, while no evidence of EGFP in ΔsigB-egfp extracts was seen with Western blotting. These findings suggest that a low level of RsbV-independent activity is present at 4°C, which is not seen at 37°C, perhaps suggesting an alternative route pathway for activation at low temperatures. The data presented above indicate that -dependent transcription at 4°C can also occur in the absence of RsbV when, according to the present model, it is expected that would be bound to RsbW and unavailable for transcription. One of the possible hypotheses suggested for a similar finding in B. subtillis was related to the instability of RsbW under nonoptimal temperature . To determine whether RsbW is degraded or its levels are diminished at 4°C Western blot analyses were performed on protein extracts from stationary phase of growth with polyclonal antibodies raised in rabbits against RsbW from L. monocytogenes EGD-e strain. Similar patterns of anti-RsbW binding were observed in wt-egfp extracts from 37°C and 4°C suggesting that temperature has no effect on RsbW degradation (Supplementary material Figure ). Furthermore, no changes in RsbW levels were recorded between wild-type and corresponding ΔsigB and ΔrsbV mutant strains grown at 4°C indicating that these deletions do not affect RsbW stability.
4.1. Activity Increases during Exponential Phase
The main aim of this study was to examine how physiological responses are coordinated in L. monocytogenes by the changes in the activity of an alternative sigma factor during growth at 37°C and at 4°C. activity was monitored by flow cytometry using cells expressing EGFP from strongly -dependent promoter (Plmo2230). The data show that within an exponentially growing population there is an increase in the proportion of cells displaying activity and this continues to increase during growth, reaching maximal activation in stationary phase where ~35% of cells have fluorescence levels above background levels at both 37°C and 4°C. Previous reports showed limited activity of in L. monocytogenes in exponential phase and the induction of -dependent expression during entry into stationary phase at 37°C [3, 28]. It was therefore somewhat unexpected to observe that the largest increase in the proportion of fluorescent cells in a population expressing EGFP from the -dependent promoter of lmo2230 occurs during exponential phase, although maximal fluorescence occurs in stationary phase. Indeed this induction of activity occurs in exponential phase at both 37°C and at 4°C. The mechanism triggering a reprogramming of the -dependent gene expression in exponential phase is unknown at present but could be related to increasing bacterial cell density. As the cells increase in number during growth the cells experience changes in the medium composition including depletion of some specific nutrients, reduced oxygen availability, medium acidification, accumulation of metabolites, and altered levels of signalling molecules. One or more of these changes could contribute to the activation of during exponential growth and further experiments will be required to identify the specific signal involved.
4.2. Activity Is Not Induced by Low Temperature in L. monocytogenes
In the present study a similar pattern of activation was observed within populations grown in cold (4°C) or optimal (37°C) temperatures. At both temperatures activity was found to be increased during exponential phase, reaching maximal levels of activity early in stationary phase (Figures 3(a) and 3(b)). These data suggest that may not play a central role during cold adaptation in L. monocytogenes. This conclusion is consistent with the findings of a number of proteomic and transcriptomic studies that have sought to define the regulon and the cold stimulon in this pathogen. Only a very limited number of genes belonging to the regulon [7, 9, 29] are also found to be present in the cold stimulon [30–32]. Of the 30 genes listed as being upregulated in both exponential and stationary phase during growth at 4°C compared to 37°C  only two (lmo1670 and lmo1937) were described before as members of regulon in one study  but not mentioned elsewhere. Furthermore, in the present study ΔsigB-egfp and ΔrsbV-egfp strains displayed comparable growth rates to the wild-type-egfp, demonstrating that activity is not critical for growth of L. monocytogenes EGD-e at low temperature in BHI. This is a conclusion that Chan and colleagues also highlighted in an earlier study . Taken together these results suggest that the modulation of activity that occurs during growth at 4°C is primarily influenced by the growth phase rather than the growth temperature.
4.3. RsbV-Independent Activation
Although the high degree of conservation between the sigB operons in B. subtilis and L. monocytogenes suggests that regulation of is similar in both organisms [12, 33], this assumption has not yet been rigorously tested in L. monocytogenes. Initial studies on the L. monocytogenes system suggest that there may be fundamental differences in how is activated in this pathogen. Firstly, environmental (physicochemical) stress and energy stress both act via RsbT in L. monocytogenes , whereas energy stress is sensed in an RsbT-independent manner in B. subtilis . More recently it has been shown that in L. monocytogenes energy stress signals can also influence activity independently of both RsbT and RsbU .
Many features of the upstream Rsb-dependent model regulating activity remain unclear in L. monocytogenes. Chaturongakul et al.  reported that RsbT contributes to activation through RsbV during exposure to both environmental and energy stresses in L. monocytogenes while in B. subtillis two separate pathways exist . A more recent study with the opuCA-lacZ reporter suggests that in L. monocytogenes induction after energy stress enters the network through an RsbT-independent pathway and that RsbU does not modulate that response . The regulon was not shown to be induced by any of the stimuli described; thus far in ΔrsbV background and both ΔrsbT and ΔrsbV showed survival reductions similar to those of the ΔsigB strain at optimal temperature . Thus, it was surprising to note that -dependent expression occurs at 4°C in ΔrsbV background when is expected to be completely inactivated by RsbW. RsbV-independent activation of has been reported for chill-stressed B. subtilis and it was also shown to be RsbU and RsbP independent . In contrast, RsbT and RsbU were shown to be required for induction in response to cold downshift from 37°C to 7°C in L. monocytogenes . Changes in the RsbW : SigB ratio at 4°C or possible chill-induced changes in RsbW functionality might contribute to the observed RsbV-independent effects on activity in the present study, but further experiments will be required to clarify this point.
In conclusion, the present study shows that L. monocytogenes cells induce activity in early exponential phase and is maximally active in the population entering the stationary phase of growth. Moreover, a similar pattern of activation is observed within populations grown in the cold and at optimal temperatures suggesting that does not play a pivotal role in cold adaptation. Finally, we demonstrate that activation can occur independently of the antisigma factor antagonist RsbV in chill-stressed cells, but the mechanism underpinning this effect requires further investigation.
Conflict of Interests
The authors declare that there is no conflict of interests regarding the publication of this paper.
The authors thank members of the Bacterial Stress Response Group and colleagues in Microbiology at NUI Galway for helpful discussions and comments. This work was supported by a Science Foundation Ireland Research Frontiers Programme Grant (no. 05/RFP/GEN0044) and by an Irish Research Council for Science, Engineering and Technology EMBARK studentship together with Thomas Crawford Hayes award to Marta Utratna, Claas Baustian and Rhodri Ceredig were supported by Science Foundation Ireland Grant no. SRC 09/SRC/B1794 and by a Science Foundation Ireland Stokes Professorship to Rhodri Ceredig.
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