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The pH-Responsive PacC Transcription Factor of Aspergillus fumigatus Governs Epithelial Entry and Tissue Invasion during Pulmonary Aspergillosis

  • Margherita Bertuzzi ,

    Contributed equally to this work with: Margherita Bertuzzi, Markus Schrettl

    Affiliation Institute for Inflammation and Repair, University of Manchester, Manchester, United Kingdom

  • Markus Schrettl ,

    Contributed equally to this work with: Margherita Bertuzzi, Markus Schrettl

    Affiliations Division of Molecular Biology/Biocenter, Medical University Innsbruck, Innsbruck, Austria, Sandoz GmbH, Kundl, Austria

  • Laura Alcazar-Fuoli,

    Affiliation National Centre for Microbiology, Instituto de Salud Carlos III, Madrid, Spain

  • Timothy C. Cairns,

    Affiliation College of Life and Environmental Sciences, University of Exeter, Exeter, United Kingdom

  • Alberto Muñoz,

    Affiliation Institute for Inflammation and Repair, University of Manchester, Manchester, United Kingdom

  • Louise A. Walker,

    Affiliation School of Medical Sciences, University of Aberdeen, Aberdeen, United Kingdom

  • Susanne Herbst,

    Affiliation Centre for Molecular Bacteriology & Infection, Imperial College London, London, United Kingdom

  • Maryam Safari,

    Affiliation Institute for Inflammation and Repair, University of Manchester, Manchester, United Kingdom

  • Angela M. Cheverton,

    Affiliation Centre for Molecular Bacteriology & Infection, Imperial College London, London, United Kingdom

  • Dan Chen,

    Affiliation Lab of Viral Diseases, National Institute of Allergy and Infectious Diseases, National Institute of Health, Bethesda, Maryland, United States of America

  • Hong Liu,

    Affiliation David Geffen School of Medicine at University of California, Los Angeles, Los Angeles Biomedical Research Institute at Harbor, University of California, Los Angeles Medical Center, Los Angeles, California, United States of America

  • Shinobu Saijo,

    Affiliation Medical Mycology Research Center, Chiba University, Chiba, Japan

  • Natalie D. Fedorova,

    Affiliation Lab of Viral Diseases, National Institute of Allergy and Infectious Diseases, National Institute of Health, Bethesda, Maryland, United States of America

  • Darius Armstrong-James,

    Affiliation Centre for Molecular Bacteriology & Infection, Imperial College London, London, United Kingdom

  • Carol A. Munro,

    Affiliation School of Medical Sciences, University of Aberdeen, Aberdeen, United Kingdom

  • Nick D. Read,

    Affiliation Institute for Inflammation and Repair, University of Manchester, Manchester, United Kingdom

  • Scott G. Filler,

    Affiliation David Geffen School of Medicine at University of California, Los Angeles, Los Angeles Biomedical Research Institute at Harbor, University of California, Los Angeles Medical Center, Los Angeles, California, United States of America

  • Eduardo A. Espeso,

    Affiliation Department of Molecular and Cellular Biology, Centro de Investigaciones Biológicas (C.S.I.C.), Madrid, Spain

  • William C. Nierman,

    Affiliation Lab of Viral Diseases, National Institute of Allergy and Infectious Diseases, National Institute of Health, Bethesda, Maryland, United States of America

  • Hubertus Haas,

    Affiliation Division of Molecular Biology/Biocenter, Medical University Innsbruck, Innsbruck, Austria

  •  [ ... ],
  • Elaine M. Bignell

    Affiliation Institute for Inflammation and Repair, University of Manchester, Manchester, United Kingdom

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The pH-Responsive PacC Transcription Factor of Aspergillus fumigatus Governs Epithelial Entry and Tissue Invasion during Pulmonary Aspergillosis

  • Margherita Bertuzzi, 
  • Markus Schrettl, 
  • Laura Alcazar-Fuoli, 
  • Timothy C. Cairns, 
  • Alberto Muñoz, 
  • Louise A. Walker, 
  • Susanne Herbst, 
  • Maryam Safari, 
  • Angela M. Cheverton, 
  • Dan Chen


18 Jun 2015: Bertuzzi M, Schrettl M, Alcazar-Fuoli L, Cairns TC, Muñoz A, et al. (2015) Correction: The pH-Responsive PacC Transcription Factor of Aspergillus fumigatus Governs Epithelial Entry and Tissue Invasion during Pulmonary Aspergillosis. PLOS Pathogens 11(6): e1004943. View correction

8 Apr 2015: The PLOS Pathogens Staff (2015) Correction: The pH-Responsive PacC Transcription Factor of Aspergillus fumigatus Governs Epithelial Entry and Tissue Invasion during Pulmonary Aspergillosis. PLOS Pathogens 11(4): e1004802. View correction


Destruction of the pulmonary epithelium is a major feature of lung diseases caused by the mould pathogen Aspergillus fumigatus. Although it is widely postulated that tissue invasion is governed by fungal proteases, A. fumigatus mutants lacking individual or multiple enzymes remain fully invasive, suggesting a concomitant requirement for other pathogenic activities during host invasion. In this study we discovered, and exploited, a novel, tissue non-invasive, phenotype in A. fumigatus mutants lacking the pH-responsive transcription factor PacC. Our study revealed a novel mode of epithelial entry, occurring in a cell wall-dependent manner prior to protease production, and via the Dectin-1 β-glucan receptor. ΔpacC mutants are defective in both contact-mediated epithelial entry and protease expression, and significantly attenuated for pathogenicity in leukopenic mice. We combined murine infection modelling, in vivo transcriptomics, and in vitro infections of human alveolar epithelia, to delineate two major, and sequentially acting, PacC-dependent processes impacting epithelial integrity in vitro and tissue invasion in the whole animal. We demonstrate that A. fumigatus spores and germlings are internalised by epithelial cells in a contact-, actin-, cell wall- and Dectin-1 dependent manner and ΔpacC mutants, which aberrantly remodel the cell wall during germinative growth, are unable to gain entry into epithelial cells, both in vitro and in vivo. We further show that PacC acts as a global transcriptional regulator of secreted molecules during growth in the leukopenic mammalian lung, and profile the full cohort of secreted gene products expressed during invasive infection. Our study reveals a combinatorial mode of tissue entry dependent upon sequential, and mechanistically distinct, perturbations of the pulmonary epithelium and demonstrates, for the first time a protective role for Dectin-1 blockade in epithelial defences. Infecting ΔpacC mutants are hypersensitive to cell wall-active antifungal agents highlighting the value of PacC signalling as a target for antifungal therapy.

Author Summary

Inhaled spores of the pathogenic mould Aspergillus fumigatus cause fungal lung infections in humans having immune defects. A. fumigatus spores germinate within the immunocompromised lung, producing invasively growing, elongated cells called hyphae. Hyphae degrade the surrounding pulmonary tissue, a process thought to be caused by secreted fungal enzymes; however, A. fumigatus mutants lacking one or more protease activities retain fully invasive phenotypes in mouse models of disease. Here we report the first discovery of a non-invasive A. fumigatus mutant, which lacks a pH-responsive transcription factor PacC. Using global transcriptional profiling of wild type and mutant isolates, and in vitro pulmonary invasion assays, we established that loss of PacC leads to a compound non-invasive phenotype characterised by deficits in both contact-mediated epithelial entry and protease expression. Consistent with an important role for epithelial entry in promoting invasive disease in mammalian tissues, PacC mutants remain surface-localised on mammalian epithelia, both in vitro and in vivo. Our study sets a new precedent for involvement of both host and pathogen activities in promoting epithelial invasion by A. fumigatus and supports a model wherein fungal protease activity acting subsequently to, or in parallel with, host-mediated epithelial entry provides the mechanistic basis for tissue invasion.


Spores of the mould pathogen Aspergillus fumigatus are agents of multiple human diseases, most of which initiate with inhalation of fungal spores and, dependent upon host immune status, compromise pulmonary integrity. Amongst the resultant diseases, invasive aspergillosis (IA) exerts the highest fatal toll, resulting globally in an estimated 200,000 deaths per annum [1]. Recipients of allogenic hematopoietic stem cell- or solid organ transplants, are particularly susceptible to IA which accounts for 43% and 19% of all invasive fungal infections in these cohorts and causes 58% and 34% mortality, respectively, at 12 weeks post-transplant [2][4]. Structural or immunological lung defects also lead to chronic, semi-invasive, pulmonary aspergillosis (CPA) having a 5 year mortality of 50% [5]. Amongst more than 200 Aspergillus species, Aspergillus fumigatus accounts for the majority of these diseases [6].

In diseases caused by A. fumigatus the initiating host-pathogen interaction occurs at pulmonary epithelia where inhaled spores can exit from dormancy, swell and generate invasive cells called hyphae, which traverse the lung epithelium. A key pathological feature of invasive- and semi-invasive aspergilloses is the destruction of the lung parenchyma, hypothesised to be governed by proteolytic enzymes secreted by the invading pathogen. Exposure of in vitro-cultured bronchial, or alveolar, epithelial cells (ECs) to fungal culture supernatants has revealed a role for fungal proteases in destruction of the mammalian F-actin cytoskeleton and loss of focal adhesion [7][9]. However, in whole animal studies of disease, it has not been possible to attribute lung damage solely to the activity of fungal proteases since A. fumigatus mutants lacking individual, or multiple, enzymes retain the ability to cause fatal invasive infections in immunocompromised hosts [9][15].

The interaction of A. fumigatus spores with alveolar epithelia can result in the internalisation of spores [16][18] but the role of this process in disease outcome remains unknown. Cells of the A549 pneumocyte cell line [18] and 16HBE14o- transformed human bronchial epithelial cells [19] internalise 30–50% of encountered spores, via an actin-dependent mechanism. Whilst the vast majority of internalised spores are killed, a small proportion (∼3%) survives and germinates inside acidic organelles [20]. This has prompted hypotheses of latent occupation of host epithelia by A. fumigatus spores, which might thereby evade host immunity and initiate disseminated infections (as reviewed by Osherov, 2011 [21]). Conversely, a curative role for epithelial activities is strongly supported by the observations of Chaudhary et al., 2012 who reported that bronchial ECs harbouring a CFTR mutation (ΔF508) demonstrate impaired uptake and killing of conidia [22]. The impact of EC-mediated activities upon disease outcomes in whole animal models of infection is presently unclear.

In fungi a conserved regulatory pathway governs the pH-dependent expression of secreted proteins and adaptation to alkaline stress [23][27]. Acting via PacC/Rim101 transcription factors, this environmental adaptation mechanism promotes the energy-efficient production of exported enzymes and metabolites, and has a demonstrated role in the pathogenicity of Candida albicans [25], [28] and Aspergillus nidulans [29]. Analysis of the transcriptomic response of invasive A. fumigatus hyphae to the mammalian pulmonary niche, identified 102 alkaline-responsive gene functions as being upregulated in leukopenic mice [30]. We therefore hypothesised that in A. fumigatus, PacC would be important for colonisation of the mildly alkaline murine lung. In this study we describe a functional genomics analysis of PacC-mediated activities which govern pathogenicity in mice. Unexpectedly, we discovered that PacC null mutants exhibit an unprecedented non-invasive phenotype, which is not an artefact of defective fungal growth, and can be recapitulated in vitro using cultured epithelia. The capacity to invade host tissues is therefore a genetically regulated trait, requiring PacC regulatory control.

In this study we exploited the differentially invasive properties of wild-type and ΔpacC isolates, to address the cellular and molecular basis of pathogen-mediated epithelial damage during Aspergillus infections. This revealed a novel mode of epithelial entry, occurring in a cell wall-dependent manner prior to protease production, and via the Dectin-1 β-glucan receptor. Our findings reveal novel mechanistic insights, having direct relevance to infection of whole animals, which will focus the onward study of A. fumigatus-mediated lung diseases upon dissecting the synergistic and/or additive impacts of temporally distinct aspects of the host-pathogen interaction at pulmonary epithelia. The multiple deficits in pathogenic activities and heightened sensitivity to echinocandin drugs, observed in ΔpacC isolates, highlight the potential of this receptor-mediated fungal signalling mechanism as a target for antifungal therapies.


The pH-responsive A. fumigatus transcription factor PacC is required for epithelial invasion and pathogenicity in leukopenic mice

To characterise the role of the A. fumigatus PacC transcription factor (AFUA_3G11970) in pathogenicity we constructed null and complemented alleles in two distinct A. fumigatus clinical isolates CEA10 and ATCC46645 (Figure S1). Relative to non-mutated isolates, PacC null mutants assumed a compact colonial phenotype on supplemented solid DMEM medium pH 7.4 (Figure 1A) which, in contrast to colonies of wild type isolates, lacked peripheral invasive hyphae, and were composed of a denser hyphal network indicative of a hyperbranching morphology (Figure 1B). This compact morphology was pH-independent, being also observed in colonies grown on Aspergillus complete medium pH 6.5 (Figure S2A), where sporulation and pigmentation of ΔpacC mutants was equivalent to that of the wild type. To assess pH sensitivity of the ΔpacC mutants we examined, on pH-buffered minimal media, the extent of radial growth at pHs 8.0 and 7.2, relative to growth at pH 6.5 (Figures S2B and S2C respectively). Consistent with a role for PacC in alkaline adaptation, ΔpacC isolates suffered growth impairment at pH 8.0, achieving approximately 10–20% of the radial growth attained at pH 6.5 (Figure S2B), compared with 40% achieved by wild-type and reconstituted strains. However, sensitivity of ΔpacC isolates to growth at pH 7.2, which approximates the pH of the mammalian lung, did not differ from that of the wild type isolates (Figure S2C).

Figure 1. Impact of pacC deletion upon A. fumigatus growth.

(A and B) Colonial growth phenotypes on supplemented DMEM, 48 hr of growth, 103 conidia. (C) Immunofluorescence-mediated visualisation of A. fumigatus growth in co-culture with A549 epithelial cells, 16 hours, supplemented DMEM pH 7.4. Fungal cells are labelled with calcoflour white and host cells are labelled with FITC-conjugated concanavalin A, 105 spores/ml, 200× magnification. (D) Quantitation of cell size (μM2) at 16 hr of co-culture with A549 cells, 104 spores/ml, growth conditions as for panel C. (E) Branching frequency of A. fumigatus hyphae, 104 spores/ml, growth conditions as for panel C.

To orchestrate alkaline adaptation, cytoplasmically localised PacC/Rim101 transcription factors must undergo pH-dependent proteolytic cleavage and nuclear entry [31]. Concordant with this model of transcription factor activation, we detected, by electrophoretic mobility shift assay (EMSA), several PacC retardation complexes, the relative quantities of which were altered under acidic and alkaline growth conditions (Figures S3A and S3B). Relative to growth at acidic pH, processed, activated forms of PacC increased in abundance upon shifting to alkaline conditions (Figures S3A and S3B). These findings are consistent with a pH-responsive mode of PacC activation, and with a conserved role for the A. fumigatus transcription factor in alkaline adaptation.

The mammalian pulmonary niche exerts multiple physiological stresses upon invading pathogens, including mildly alkaline pH, hypoxia, and iron-, zinc- and nutrient limitation [30], [32], [33]. To compare the growth rates of wild type and ΔpacC hyphae in a physiologically relevant setting, we devised an in vitro epithelial infection assay (Figure 1C), comprising monolayers of A549 alveolar epithelial cells cultured in supplemented DMEM medium (pH 7.4). We used this assay to assess the growth rates of wild type and ΔpacC isolates, under 5% CO2 (Figure 1C). To promote the visualisation of, and distinction between, fungal and host cells we stained host cells with FITC-labelled concavalin A and fungal cells with calcofluor white. We then performed a quantitative analysis of fungal growth rate (Figure 1D) and hyphal branching (Figure 1E) via immunofluorescence microscopy. Inspection of the infected monolayers revealed significant hyphal growth of both wild type and ΔpacC isolates (Figure 1C), but quantitation of hyphal branching frequency revealed an approximately doubled frequency of hyphal branching amongst ΔpacC isolates relative to wild type. To normalise for heightened branching during quantitation of hyphal growth rates we performed a comparative assessment of individual cell sizes by enumerating the number of pixels per fungal particle. This analysis, revealed that the cross-sectional area of wild type and ΔpacC cells approximates 540 versus 387 µm2 respectively (Figure 1D) which, assuming a uniform hyphal radius for wild type and mutant cells of approximately 3 µm, equates to a maximum deviance of 20 µm in length after 16 hours of in vitro co-culture with mammalian epithelia. On this mathematical basis, the median length of an unbranched ΔpacC hypha would be ∼ 30 µm. Given that ∼ 50% of ΔpacC hyphae remain unbranched, and the thickness of the alveolar epithelium is comparatively tiny, the observed differences in hyphal length between wild type and mutant hyphae are insufficient to explain the non-invasive phenotype of the ΔpacC mutants.

Leukopenia is an important risk factor for IA in humans, and cyclophosphamide-induced leukocyte depletion renders mice highly susceptible to pulmonary infection [34]. To assess the role of A. fumigatus PacC in pathogenicity we assessed the survival of leukopenic mice following infection, via the intranasal route, with spores of wild-type, ΔpacC or reconstituted isolates (Figure 2A). Relative to wild-type strains, ΔpacCATCC and ΔpacCCEA10 mutants were significantly attenuated for virulence (Figure 2A). At day 6 post-infection 100% of mice infected with the ΔpacC mutants remained alive while 78% and 92% of mice infected with wild type (ATCC46645 and CEA10 respectively) isolates were dead.

Figure 2. PacC is required for pathogenicity and epithelial invasion in leukopenic mice.

(A) Kaplan-Meier curve for murine survival (n ≥ 9) after infection with 6 × 105 and 5 × 104 spores for ATCC46645 and CEA10 respectively. (B) Histopathology of leukopenic murine lungs after 4, 8, 12, hr of infection with ATCC46645 and ΔpacCATCC (108 spores), Grocott's Methenamine silver (GMS) and light green staining, 200× magnification. (C) ΔpacCATCC hyphae (black arrows) are unable to penetrate the respiratory epithelium (RE), BA indicates bronchial airway space, 20 hr post-infection, 400× magnification.

Histological analysis of infected lung tissues revealed significant differences between mutant and wild-type isolates by 20 hours post-infection (Figures 2B and C). While ΔpacC spores appeared to swell and form primary germ tubes by 12 hours post-infection (Figure 2B), penetration of the lung epithelium was not evident and, despite being competent in hyphal production in the murine airway, ΔpacC germlings remain contained within the epithelial boundary of the airspace at 20 hours post-infection (Figure 2C). Thus, ΔpacC germlings in leukopenic hosts exhibited a marked tissue non-invasive phenotype (Figures 2B and 2C).

To further characterise the non-invasive phenotype of ΔpacC isolates we used our in vitro co-culture assay (Figure 1C) to examine integrity of A549 alveolar epithelial monolayers following 16 hours co-culture with wild-type or ΔpacC isolates by enumeration of detaching epithelial cells. In monolayers infected with wild-type strains, extensive rounding and detachment of up to 40% of host cells was demonstrable, resulting in observable destruction of the epithelial monolayer (Figures 1C and 3A). However, similar to PBS-challenged monolayers, infection with ΔpacC mutants led to detachment of less than 5% of monolayer cells (Figures 1C and 3A). Although ΔpacC hyphae achieved similar hyphal growth rates (Figure 1D) and epithelial coverage (Figure 1C) to isogenic wild type isolates, ΔpacC hyphae were found to navigate the surface of the epithelial monolayer without effecting cellular detachment (Figure 1C).

Figure 3. Quantitative analysis of epithelial integrity.

(A) Percent detachment, relative to PBS challenge, quantified from a similar experiment as that depicted in Figure 1C. Significance was calculated relative to PBS-challenged A549 cells. (B) Quantification of A549 damage by 51Cr release assay upon infection with A. fumigatus (5 × 105 spores/ml) for 16, 20 and 24 hr. A and B: technical and biological triplicate, unpaired t test. *** p<0.001, ** 0.001 <p<0.01, and * 0.01 <p<0.05.

To further characterise this deficit in epithelial damage, a modified 51Cr release assay [35], adopting a similar time course of infection, was utilised to quantitatively assess epithelial cell lysis upon infection (Figure 3B). Concordant with cell detachment assays, ΔpacC mutants reproducibly failed to fully elicit epithelial damage. Taken together these findings demonstrate that ΔpacC hyphae fail to elicit disintegration of alveolar epithelia during in vitro culture at pH 7.4 despite achieving similar growth rates as wild-type isolates (Figures 1C and D and 3A and B).

Several observations argue strongly against a trivial pH-dependent growth defect as the basis for the ΔpacC virulence defect. First, in A. fumigatus, a compact colonial morphology is not a robust correlate of reduced virulence. For example, despite compact colonial morphology and a highly branching mode of growth, null mutants lacking the ChsG chitin synthase remain fully virulent in an inhalational model of infection [36]. Second, in A. fumigatus, in vitro alkaline sensitivity is not a robust correlate of reduced virulence. For example, mutants lacking the mitogen-activated kinase MpkA, demonstrate more severe radial growth defects than ΔpacC mutants in Aspergillus minimal medium [37] and exhibit highly alkaline sensitive phenotypes [38], but retain full virulence in a low dose inhalational model of aspergillosis. Third, during in vitro cell culture with A549 cells (pH 7.4), hyphae of ΔpacC mutants achieve similar growth rates to that of isogenic wild type isolates (Figures 1C and D). Fourth, despite achieving similar growth rates to wild type hyphae during in vitro cell culture with A549 cells (pH 7.4), hyphae of ΔpacC mutants fail to elicit epithelial decay (Figures 1C, 3A and B). Finally, hyphae of ΔpacC mutants fail to traverse the murine epithelium and are strictly confined to the airway (Figure 2C). ΔpacC mutants are the first-reported non-invasive A. fumigatus mutants, revealing that tissue invasion is a genetically regulated trait under PacC regulatory control. We therefore exploited the differentially invasive properties of wild type and ΔpacC isolates to seek a more detailed mechanistic understanding of tissue invasive growth in this pathogen.

PacC modulates expression of genes encoding secreted enzymes and cell wall- and gliotoxin biosynthetic activities during invasive aspergillosis

Previously, we devised a strategy for analysing A. fumigatus gene expression during initiation of murine aspergillosis [30]. Here we applied a similar approach, this time performing time-series analyses (4, 8, 12 and 16 hours) of A. fumigatus gene expression. This permitted the capture of stage-specific gene expression during invasive colonisation of the leukopenic murine lung, the first reported longitudinal study of gene expression during mammalian pulmonary infection. We adopted a comprehensive experimental design (Figure S4A), incorporating 12 competitive hybridisations and 12 flip-dye experiments. This permitted the analysis of stage-specific gene expression in both infecting wild-type ATCC46645 (Figure S4B) and ΔpacCATCC isolates (Figure S4C), as well as the directly comparative analysis of gene expression, by time-point, for the wild type and ΔpacCATCC mutants (Figure S4D).

Relative to ungerminated spores, transcript profiling of wild-type gene expression revealed a total of 3733 genes, (log2≥ +/−1.5), which were differentially expressed at a minimum of one time-point during invasive infection. The differentially regulated genes were assigned to three cohorts, corresponding to (i) genes consistently up- or down-regulated across the time series; or differentially regulated during (ii) early (4, 8 and 12 hours) or (iii) late (12 and 16 hours) phases (Dataset S1). This revealed respiration, metabolism and amino acid biosynthesis as being prioritised during early infection of the leukopenic host, while cation transport, secondary metabolism and iron metabolism were subsequently emphasised during commencement of invasive growth (Dataset S1). Throughout the time series of growth in the host, upregulated expression of secreted gene products remained highly significant. A comprehensive functional, and statistical, analysis of differentially regulated gene products is provided in Dataset S1.

Directly comparative analysis of ΔpacCATCC and ATCC46645 activities (Dataset S2) revealed 1116 genes to be differentially expressed. Of these, 577 were up-regulated and 539 were down-regulated in the ΔpacCATCC isolate, relative to the wild type isolate, in at least one time point of the analysis. Scrutiny of the datasets revealed dysregulated expression of secreted protein gene products, defined as having predicted signal peptide motifs (Figure S5), cell wall biosynthetic enzymes (Figure S6), and gliotoxin biosynthetic genes (Figure S7) during infections caused by the ΔpacCATCC isolate. A comprehensive functional, and statistical, analysis of differentially regulated gene products is provided in Dataset S2. The differential regulation of 5 genes was independently validated by quantitative PCR (Figure S8).

A. fumigatus perturbs epithelial integrity via distinct, and sequentially implemented, mechanisms which are defective in ΔpacC isolates

A. fumigatus spores adhere rapidly (within 30 minutes) to lung pneumocytes and become quickly internalised and killed [16][18], [20]. In response to challenge with A. fumigatus conidia, host injury can be observed as cell rounding and detachment from monolayers [16][18], [20], and cytoskeletal fibres of lung pneumocytes suffer major reorganisation, an effect which can be blocked by antipain-mediated protease inhibition [8]. We found secreted factors to be the major functional cohort amongst those aberrantly regulated during ΔpacC infections (Figure S5, and Dataset S2). To assess the role of secreted factors in epithelial disintegration we exposed A549 monolayers to A. fumigatus culture filtrates derived from young (16 hours), or mature (48 hours), wild-type or ΔpacC cultures grown in supplemented DMEM culture medium. Filtrates obtained from mature cultures of wild-type or reconstituted A. fumigatus isolates, prompted significant reductions (∼30–40%) in the numbers of adherent cells after 20 hours of co-incubation with alveolar epithelia (Figure 4A). In contrast, filtrates derived from mature ΔpacC cultures led to detachment of less than 10% of monolayer cells (Figure 4A). Concordant with a protease-mediated basis for epithelial destruction, pre-treatment of wild-type A. fumigatus culture filtrates with the protease inhibitor antipain [8] reduced cellular detachment by up to 50% (Figure 4A). To further probe protease production by wild type and mutant isolates, we used a qualitative assay based upon the clearance of gelatin from the surface of unprocessed X-ray film [39]. In agreement with our assays of epithelial degradation (Figure 4A) we detected gelatin-degrading activity in filtrates of mature wild type and reconstituted A. fumigatus cultures, which was absent in cultures from ΔpacC isolates (Figure S9).

Figure 4. Distinct and sequential PacC-dependent activities elicit epithelial decay.

(A) Percent detachment, relative to PBS challenge, of A549 cells exposed to antipain-treated and non-treated fungal culture supernatants (48 hr cultures, 105 spores/ml). (B) Integrity of A549 monolayers following exposure to fungal culture supernatants (16 hr cultures, 105 spores/ml). 200× magnification. (C) Percent aberrant morphology, amongst fungus-proximal ECs, per unit of hyphal length, relative to wild-type challenged monolayers. Monolayers were incubated for 18 hr or 36 hr (ΔpacC mutants). A and B: technical and biological triplicates and C: performed twice in triplicate, 1-way ANOVA test, *** p<0.001 and ** 0.001 <p<0.01.

Together, these findings are consistent with the release of a damaging proteolytic entity by mature A. fumigatus hyphae, the production of which is dependent upon PacC-mediated signalling. Notably, epithelia challenged with ΔpacC culture supernatants were somewhat protected by pretreatment of fungal extracts with antipain (Figure 4A). This might indicate the production of a protective, host-derived enzyme which is degraded or inactivated by culture filtrates of wild type A. fumigatus isolates, or the existence of a protective, host-derived enzyme whose action, in this assay, is masked by the high degree of epithelial detachment imposed by wild type isolates.

Critically, our analysis of filtrates obtained from younger fungal cultures (16 hours) revealed a novel finding. Regardless of the fungal strain tested, exposure to filtrates from young cultures did not impact monolayer integrity (Figure 4B). This finding suggested that epithelial disintegration occurring at 16 hours of spore and EC co-incubation (Figure 4B) requires direct interaction between host and pathogen cells and represents a genetically regulated fungal assault upon epithelial integrity which is temporally, and mechanistically distinct from protease-mediated damage. Further, that this damaging interaction between host and pathogen cells occurs during immediate proximity between host and pathogen cells, most likely in a contact-dependent manner. To substantiate this view we reiterated the detachment analysis, this time omitting monolayer washing to analyse only host cells directly contacting the pathogen (Figure 4C). A549 cells in contact with ΔpacC hyphae underwent significantly less rounding and detachment than those contacting hyphae of wild-type or reconstituted isolates (Figure 4C). Taken together, these data reveal that A. fumigatus elicits host damage in a biphasic manner and, that the pH-responsive transcription factor PacC governs functions required for epithelial disintegration during both early- and late-phases of the host-pathogen interaction.

A. fumigatus causes epithelial disintegration in a cell wall-dependent manner

Amongst the functional cohorts aberrantly regulated during ΔpacCATCC infections (Figures S5S7 and Dataset S2) cell wall biosynthesis offered a plausible mechanism for contact-dependent host damage. To analyse cell wall compositions of mutant and wild-type isolates, strains were stained with the chitin-binding agent calcofluor white (CFW). Microscopic examination revealed intensified CFW-staining of ΔpacC germ tube tips relative to those of the parental isolates (Figure 5A) and quantitative analysis of fluorescence intensities revealed significantly higher CFW in ΔpacC germ tubes (Figure 5B). In addition, electron microscopy showed a thickened cell wall in the ΔpacCATCC mutant, which was highly evident after 16 hours of growth (Figure S10). Hyphal cell wall composition (Figures 5C, D and E) was assessed by high-performance anion exchange chromatography with pulsed amperometric detection (HPAEC-PAD). After 16 hours of growth, cell wall chitin content was found to be 20% higher in extracts from ΔpacC isolates, relative to wild-type cells (Figure 5C). The quantity of cell wall glucan and mannan was measured as equivalent between mutant and wild type cells (Figures 5D and 5E).

Figure 5. Aberrant morphology of A. fumigatus ΔpacC mutants impacts contact-mediated epithelial decay.

(A) Calcofluor white staining of A. fumigatus strains after growth for 17–18 hr in AMM (pH 6.5) at 28°C. (B) Quantification of calcofluor white-mediated fluorescence (arbitrary units) as measured from panel A. (C) Percentage, in cell wall extracts relative to total weight, of chitin. (D) Percentage, in cell wall extracts relative to total weight, of glucan. (E) Percentage, in cell wall extracts relative to total weight, of mannan. (F) Percent detachment, relative to PBS challenge, of A549 cells after co-incubation with cell wall extracts (10 µg/ml). Significance was calculated relative to PBS-challenged monolayers. (G) Percent aberrant morphology, amongst thimerosal-killed fungus-proximal ECs, per unit of hyphal length, relative to wild-type challenged monolayers. B and C: biological and technical triplicates. D and E: performed twice in triplicate. B, C and D: unpaired t test. E: 1-way ANOVA test. *** p<0.001 and ** 0.001<p<0.01.

To probe the contribution of cell wall components to epithelial cell detachment, we exposed A549 monolayers to cell wall extracts. This revealed that, relative to the vehicle control, the percentage of adherent cells was drastically reduced upon exposure to cell wall extracts from wild-type isolates, an effect which was not elicited by ΔpacC cell wall extracts (Figure 5F).

If detachment of alveolar epithelial cells occurs via a cell wall-mediated mechanism, infection with dead hyphae would be predicted also to cause cellular detachment. To test this, A549 monolayers were incubated with thimerosal-killed hyphae and cell detachment, per unit of hyphal length, was measured from unwashed monolayers. Killed hyphae from parental isolates caused damage to the epithelial monolayer independently of fungal viability, an effect which was significantly impaired in monolayers incubated with killed ΔpacC hyphae (Figure 5G). In conclusion, epithelial detachment elicited early in the interaction between A. fumigatus and host cells requires contact between host and pathogen and occurs independently of fungal viability. Crucially, the inability of killed ΔpacC hyphae to injure epithelial monolayers eliminated the trivial possibility that mere collision between host and fungal cells can account for loss of monolayer integrity.

Dectin-1, in alveolar epithelial cells, promotes internalisation of A. fumigatus spores

The mammalian C-type lectin receptor Dectin-1, is predominantly expressed by myeloid cells and recognizes a variety of fungal β-1,3-linked and β-1,6-linked glucans [40][42]. Recent transcriptional and immunohistochemical analyses have revealed Dectin-1 gene expression in bronchiolar epithelia, and alveolar type II cells (ATIIs) of murine lungs [43] and Han et al., showed that A549 cells internalise germinated A. fumigatus spores in a phospholipase D-dependent manner, a process inhibited by an anti-Dectin-1 antibody [44]. Given these observations and aberrant cell wall remodelling in (Figure 5), and epithelial damage by (Figure 4), ΔpacC mutants we hypothesised non- or reduced involvement of Dectin-1 in promoting A. fumigatus ΔpacC spore recognition and internalisation.

Epithelial cells have been shown to internalise and kill up to 50% of the A. fumigatus spores they come into contact with [16][19], [22]. We therefore hypothesised that contact-dependent perturbations of epithelial integrity might result from internalisation of fungal spores. To assess this we first assessed the numbers of internalised wild type and ΔpacC spores using a nystatin protection assay (Figure 6A). This revealed that the proportion of wild-type spores internalised by A549 cells ranges from 16 to 23% (Figure 6A). However, epithelial cells were found to internalise ΔpacC mutants significantly less avidly than the respective parental isolates (Figure 6A), whereby only ∼10–12% of the initial inoculum had become internalised after 4 hours of co-incubation. At the concentrations used in this assay nystatin exposure was 100% efficient in killing A. fumigatus spores (Figure S11).

Figure 6. ΔpacC mutants are less avidly internalised by A549 and spore internalisation depends on Dectin-1.

(A) Percent internalisation by nystatin protection assay. Epithelial monolayers were incubated with 106 spores/ml for 4 hr, n  =  9 for wild types and ΔpacC. (B) Percent internalisation, when blocking the Dectin-1 receptor (0.3 µg/ml α-Dectin-1 antibody) or actin-mediated internalisation (0.2 µM CD), or in the presence of an isotype control antibody (0.3 µg/ml) technical and biological duplicates. (C) Percent detachment, relative to PBS challenge, of A549 upon infection with A. fumigatus (105 spores/ml) for 16 hr and inhibition of actin-mediated internalisation via Cytochalasin D (CD, 0.2 µM), when blocking the Dectin-1 receptor (0.3 µg/ml α-Dectin-1 antibody) or in the presence of an isotype control antibody (0.3 µg/ml), technical and biological triplicates. (D) Use of a soluble Fc Dectin-1 protein for immunofluorescence-mediated imaging of β-glucan in A. fumigatus spores, 4 hr, supplemented DMEM. (E) A. fumigatus spore size (μM2), 4 hr, supplemented DMEM. A, B, C: unpaired t test (unless otherwise indicated) *** p<0.001, ** 0.001<p<0.01, and * 0.01<p<0.05.

Given the altered cell wall morphology of ΔpacC isolates a plausible explanation for their defective internalisation might include an adhesion defect. We therefore tested the ability of the isolates to adhere to plastic surfaces and epithelial monolayers after 30 minutes of incubation. However, for neither substrate was a difference in adherence observed, either for the ΔpacC mutants or wild type isolates (Figure S12). Taken together, these data suggest that internalisation of A. fumigatus spores, which is hampered by pacC deletion, contributes to contact-dependent monolayer decay.

To assess the role of Dectin-1 in promoting epithelial decay in vitro we pre-incubated epithelial cells with the monoclonal anti-Dectin-1 antibody (Mab1859) prior to performing nystatin protection assays. Concordant with a role for Dectin-1 in spore internalisation, epithelial monolayers pre-treated with Mab1859 exhibited a ∼20–30% reduction in internalised spores, relative to untreated epithelia (Figure 6B). As a control we used 0.2 µM cytochalasin D (CD), an inhibitor of actin polymerization, which prevents spore internalisation into A549 cells [18]. The impact of CD treatment (50% reduction) was consistently greater than that of Mab1859, possibly indicating the contribution of additional spore-detecting PRRs driving spore internalisation and/or opsonic phagocytosis and/or incomplete Mab1859-mediated inhibition of Dectin-1 activity.

To assess the impact of spore internalisation upon epithelial integrity, A549 monolayers were pre-treated for 1 hour with CD and detachment after 16 hours was evaluated using our in vitro assay. For wild type infections, cellular detachment from epithelial monolayers was significantly reduced from ∼45% to ∼25% in the presence of CD (Figure 6C) but pre-incubation with CD did not alter integrity of ΔpacC-challenged monolayers (Figure 6C). These results suggested that actin-mediated internalisation of wild-type spores contributes to epithelial detachment during initial interactions with fungal spores.

To further probe the molecular basis of epithelial decay, monolayers were preincubated with the monoclonal anti-Dectin-1 antibody (Mab1859) prior to co-incubation with A. fumigatus spores. Concordant with a damaging role for Dectin-1 mediated internalisation of A. fumigatus spores and hyphae in A549 alveolar monolayers, Mab1859 pre-treatment conveyed an almost complete protection of monolayer integrity during co-incubation with wild type A. fumigatus isolates (Figure 6C).

To characterise the cell wall defect inhibiting Dectin-1-mediated uptake of ΔpacC we examined β-glucan content in the cell walls of wild type and ΔpacC spores and hyphae, by incubating fungal cells with a soluble chimeric Dectin-1 Fc protein [45], [46] and quantifying immunofluorescence. This revealed highly anomolous organisation of β-glucan content in ΔpacC spores (Figure 6D). Relative to wild type spores which deposit β-glucan at a highly localised, and singular focus of the spore cell wall prior to germination, β-glucan in ΔpacC spores adopts a highly diffuse distribution. This phenotype is not a consequence of slowed spore swelling as wild type and ΔpacC spores demonstrate equivalent sizes at 4 hours of culture in supplemented DMEM (Figure 6E).

In Histoplasma capsulatum α-1,3-glucan promotes virulence by blocking innate immune recognition of β-glucan by Dectin-1. To examine α-1,3-glucan content in A. fumigatus spores and hyphae we used immunofluorescence microscopy and anti-α-1,3-glucan antibody, which has previously been used for analysis of the H. capsulatum cell wall [47]. Immunofluorescence-mediated detection of this antibody revealed similar distributions of α-glucan in wild type and ΔpacC hyphae (Figure S13).

Taken together these data support an important role for internalisation of A. fumigatus spores during invasion of the pulmonary epithelium which, in a cell wall-, actin- and Dectin-1 dependent manner permits endocytosis of fungal particles contacting alveolar epithelia.

Dectin-1 protects murine pulmonary epithelia from A. fumigatus-mediated damage

The extent of epithelial protection afforded by in vitro delivery of Mab1859 (Figures 6B and C) was suggestive of a detrimental role for Dectin-1 engagement during A. fumigatus-epithelial interactions. To decipher between protective and exacerbatory roles for Dectin-1 in maintenance of epithelial integrity in whole animals, we assessed pulmonary damage after 24 hours of A. fumigatus infection in Dectin-1+/+ and Dectin-1−/− mice. To study epithelial activities in the absence of confounding leukocyte responses, mice were depleted of leukocytes using a cyclophosphamide and hydrocortisone protocol and lung injury was scored via histological, biochemical and immunoblot assays. In the lungs of Dectin-1+/+ and Dectin-1−/− mice, fungal lesions were equivalent in size and invasiveness (Figure 7A) although frequency of fungal lesions was increased in Dectin-1−/− animals (not shown). Epithelial damage was surveyed via quantitation of lactate dehydrogenase (LDH) in BALs (Figure 7B) and analysis of expression of the Dectin-1-independent damage associated molecular pattern (DAMP) protein S100B (Figure 7C), whose major source during A. fumigatus infection is epithelial cells [48]. Both assays revealed heightened epithelial damage in the lungs of Dectin-1−/− animals relative to wild type counterparts. Our results indicate that, despite a highly protective role for the anti Dectin-1 antibody Mab1859 during in vitro epithelial infections, integrity of Dectin-1 (Figures 7A–C) is essential for limitation of epithelial damage in vivo. As neutrophil-depletion and macrophage dysfunction were chemotherapeutically implemented in our murine model we conclude that Dectin-1 activity is essential for protecting the lung epithelium from the damage inflicted by germinating A. fumigatus spores.

Figure 7. Internalisation and Dectin-1 protect murine pulmonary epithelia from A. fumigatus-mediated damage.

(A) Histopathology of Dectin-1−/− and Dectin-1+/+ leukopenic mice (n  =  3) infected with CEA10 (108 spores, 24 hr of infection, GMS and light green staining, 200× magnification). (B) LDH/BCA fold change in BALs from Dectin-1−/− and Dectin-1+/+ leukopenic mice (n  =  3) infected as in B, technical triplicates. (C) S100B western blotting on lung homogenates from Dectin-1−/− and Dectin-1+/+ leukopenic mice infected as in B. Densitometry plot where pooled densitometry values for S100B were normalised on pooled densitometry values for actin and background subtracted for the saline controls. (D) Macrophages and neutrophils (cells/ml) in BALs from immunocompetent mice infected with ΔpacCCEA10 mutant and CEA10 (n  =  4, 106 spores, 24 hr of infection). B and C: unpaired t test, *** p<0.001 and * 0.01<p<0.05.

PacC homologues in the fungal pathogens C. albicans and Cryptococcus neoformans indirectly modulate interactions with the host interface via governance of fungal cell wall architecture. For both organisms, cell surface defects in Rim101 null mutants appear to be a critical component of altered pathogenicity. In C. albicans, oropharyngeal pathogenicity, estimated from in vitro assessment of damage in the FaDu cell line, can be partially restored to attenuated Rim101 null mutants via overexpression of the Rim101 target genes ALS3, CHT2, PGA7/RBT6, SKN1 or ZRT1 [49]. In C. neoformans Rim101 null mutants, via cell wall defects, prompt aberrant inflammatory responses, resulting in mild hypervirulence [50]. Thus, in the case of both organisms, host immune responses to altered cell wall composition play a functional role in disease outcome. To test the immunostimulatory capacity of wild-type and ΔpacC spores, immunocompetent CD1 mice were infected with 106 spores and the recruitment of macrophages (F4/80+) and neutrophils (Ly-6G+) to the pulmonary niche was quantified. Relative to mice infected with a wild-type isolate, no significant difference in the number of recruited neutrophils was recorded for mice infected with the ΔpacC mutant (Figure 7D). Further, and in stark contrast to findings in C. neoformans, we did not observe (in immunocompetent hosts) a hyperinflammatory response to infection with ΔpacC mutants. We therefore conclude that anomalous innate immune responses are unlikely to contribute to the altered pathogenicity of A. fumigatus ΔpacC mutants. Therefore, in stark contrast to oral and pulmonary infections, respectively with C. albicans [49] and C. neoformans [50][52], modulation of host innate immunity is unlikely to contribute to A. fumigatus disease outcome.

Taken together our results indicate that the predominant host-mediated mechanism promoting the non-invasive phenotype of A. fumigatus ΔpacC mutants is a failure to engage the Dectin-1 receptor. It is therefore highly likely that A. fumigatus exploits this innate immune mechanism to gain entry to the pulmonary epithelium. The important role for Dectin-1 in epithelial protection in vivo implies that the full extent of systemic Dectin-1 depletion upon epithelial defences likely extends well beyond defective internalisation of inhaled fungal spores. However, given the propensity of A. fumigatus to exploit this mode of tissue entry, it remains possible that the targeted depletion of epithelial Dectin-1 activity would afford protection against invasive, and other, A. fumigatus diseases of the lung.

ΔpacC mutants are hypersensitive to cell wall active drugs

The fungal cell wall is a premier, pathogen-specific target for antifungal drugs. Given the significant cell wall defect observed in ΔpacC mutants we predicted altered echinocandin sensitivity relative to wild type isolates. A standard EUCAST assay [53] was used to calculate the susceptibility of isolates, revealing increased susceptibility (Figure 8A) of ΔpacC mutants (minimum effective concentration, MEC, of 0.11 µg/ml) compared to that of ATCC46645 (∼ 0.58 µg/ml) and CEA10 (∼ 0.75 µg/ml). A. fumigatus strains grown in the presence of 16 µg/ml caspofungin displayed aberrant morphology, elevated branching and shortening of hyphae. Heightened severity of these phenotypes was observed for ΔpacC mutants which demonstrated extensive ballooning of hyphal tips (Figure 8B). Given the tendency for chitin increase to promote echinocandin tolerance the heightened susceptibility of ΔpacC mutants is surprising; however, an obvious explanation for this effect would be increased porosity due to altered cell wall architecture.

Figure 8. ΔpacC mutants are hypersensitive to cell wall active drugs.

(A) In vitro susceptibility testing to caspofungin (CFN). Determination of CFN MEC (μg/ml), twice in triplicates, 1.25 × 105 spores, 48 hr. (B) A. fumigatus growth in the presence of 16 µg/ml CFN. 400× magnification. (C) Histopathology from leukopenic mice infected with CEA10 or ΔpacCCEA10 (3 × 104 spores) in the presence or absence of 5 mg/kg CFN. Lungs sections at 24 hr of infection, GMS and light green staining, 200× magnification. (D) In vivo susceptibility testing to caspofungin. Fungal burden at 48 hr of infection, calculated by CFUs, from leukopenic mice infected as from C. Results are expressed as CFUs per gram of lung tissue. A and D: unpaired t test, *** p<0.001, **.001<p<0.01, and * 0.01<p<0.05.

To test the potency of echinocandin agents against pH non-sensing mutants in vivo we examined, via viable counts, the effect of caspofungin (5 mg/kg) treatment at 48 hr post-infection. Relative to animals infected with a wild type isolate, fungal burden was significantly decreased in caspofungin-treated mice infected with ΔpacCCEA10 (Figure 8C). Histological analysis of lung tissues recovered from mice infected with CEA10 or ΔpacCCEA10 in the presence or absence of caspofungin confirmed this observation (Figure 8D). Thus, ΔpacC mutants are hypersensitive to the cell wall-active drug caspofungin, a phenotype which extrapolates to mammalian infections (Figures 8C and 8D). Given that the A. fumigatus cell wall is essential for viability, agents which selectively inhibit the pH-dependent activation of PacC signalling might provide useful adjuncts to existing antifungal therapies.


Amongst an annual global caseload of 1.5 million fatal mycoses, more than 75% of infections are initiated by inhalation of fungal particles [1]. Despite this, our understanding of the interactions between inhaled fungal pathogens and the respiratory epithelium remains in its infancy. This study addresses disease caused by the major mould pathogen of humans, A. fumigatus, and assigns an essential role for the transcription factor PacC in epithelial invasion and pathogenicity. A critical discovery made during this study is the inability of ΔpacC mutants to invade the mammalian respiratory epithelium, a hallmark of invasive diseases caused by A. fumigatus. Our study confirms that epithelial invasion by this pathogen is a genetically-regulated trait, under PacC regulatory control, and identifies the cellular basis of the deficit to lie with at least two temporally and mechanistically distinct processes, namely protease-mediated monolayer decay and epithelial entry.

Compared to our previous studies of A. nidulans pH regulation [29], loss of A. fumigatus PacC has a milder impact on alkaline tolerance and in vivo germination. At least one mode of essential micronutrient acquisition is different between the two species. In A. nidulans, siderophore-mediated iron acquisition is PacC-dependent [54], in A. fumigatus it is not (Hubertus Haas personal communication). Certainly this could explain the differences between these two species in germination/growth rates in the mammalian lung.

The A. fumigatus genome is predicted to encode more than 100 hydrolytic enzymes [55] some of which are assumed as crucial for liberation of proteinaceous nutrients from host tissues [56], [57]. Early studies found a correlation between high elastinolytic potency of A. fumigatus isolates and pathogenicity in mice [58] but a subsequent survey of 73 isolates revealed discordant production of extracellular elastase, acid proteinase and phospholipase amongst strains causing human disease. The elastinolytic neutral metalloprotease Mep (AFUA_8G07080), secreted in A. fumigatus culture filtrates and leukopenic murine hosts [59], is dispensable for pathogenicity.

A. fumigatus culture filtrates cause epithelial desquamation and destroy F-actin cytoskeletal fibres of in vitro-cultured pneumocytes [8], [60]. Kogan et al., 2004 found deletion of the alp1 gene (AFUA_4G11800) encoding a secreted alkaline protease, or antipain treatment of wild-type culture supernatants to be equally ablative of secreted protease activity in vitro. In addition, immunolabelling of the F-actin cytoskeletal fibres of A549 cells revealed that F-actin disruption requires Alp1 integrity. However, an A. fumigatus mutant lacking Alp1 retained full virulence in both cortisone-treated [61] and leukopenic mice [15]. Attempts to implement wholesale depletion of A. fumigatus protease expression have also failed to unearth avirulent mutants. A doubly protease-deficient mutant lacking Alp1 and Mep, which is completely deficient in collagenic proteolytic activity at neutral pH in vitro, is fully virulent in a cortisone-treated murine model [13]. Furthermore, an A. fumigatus ΔprtT mutant lacking a conserved positive regulator of secreted proteases suffers a 70% reduction in casein proteolytic activity, but is also fully virulent in leukopenic mice. These findings cast doubt upon the true relevance of protease production to A. fumigatus pathogenicity [10]. Comparison of the PacC and PrtT [9] regulons revealed 83 and 31 secreted gene products as being down-regulated by PacC and PrtT (AFUA_4G10120) respectively, amongst which only 8 are commonly down-regulated (Dataset S3). Given the fully virulent phenotype of the ΔprtT, mutant we can confidently surmise that none of these gene products, acting alone or in combination with each other, can support tissue-invasive growth in the mammalian host. Thus their aberrant expression in the ΔpacC mutant is unlikely to explain its non-invasive phenotype. Concordant with this conclusion, and with the fully virulent phenotype of a Δmep;Δalp1 mutant [13], the inclusion of genes encoding both Alp1 and Mep1 (Dataset S3) amongst those down-regulated in both PacC and PrtT null mutants cannot, alone, explain the non-invasive phenotype of PacC null mutants. Loss of PacC negatively impacts a further 75 uncharacterised secreted gene products. If the tissue invasive growth of A. fumigatus is solely proteolytically mediated, we predict that important enzymatic functions will be amongst them. Investigation of this hypothesis lies beyond the scope of this study but is an ongoing component of our further study, as is the co-operative activity of fungal protease- and toxin-mediated assaults upon the mammalian pulmonary epithelium.

The finding that epithelial monolayers are resistant to culture filtrates obtained from earlier (16 hour) time points of fungal growth highlights the existence of at least one additional, and earlier acting, perturbation of host tissue. Soluble effectors of epithelial detachment are not immediately secreted by metabolically active A. fumigatus spores and a phased mode of A. fumigatus assault, commencing with contact-dependent perturbation, is likely responsible for monolayer perturbation. In agreement with this hypothesis, we found cytochalasin D-mediated inhibition of actin polymerisation to be partially protective of epithelial monolayer integrity, and ΔpacC spores to be far less avidly internalised than wild-type counterparts. Amongst the repertoire of invasion tactics employed by fungal pathogens at host epithelia, induced endocytosis, active penetration and participation of host factors have been implicated [52]. The results of our study implicate all three activities as having relevance to the host-A. fumigatus interaction, but with several critical differences relative to studies of other fungal pathogens. Firstly, the occurrence of induced endocytosis, as evidenced by sensitivity of the internalisation process to cytochalasin D-mediated inhibition (Figure 6C), promotes epithelial disintegration by both live and dead fungal elements. This finding stands in stark contrast to epithelial invasion by C. albicans where internalisation of live germinated cells, but not killed cells, leads to host damage [62]. Second, the existence of A. fumigatus invasins remains thus far unproven. Certainly, from bioinformatics analyses, evidence for highly conserved homologues for the C. albicans invasin Ssa1 can be gleaned. However the expression of this homologue is not impacted by pacC gene deletion and A. fumigatus lacks any homologue of the Als3 invasin altogether [63], [64]. Our finding that cell wall extracts can impact epithelial integrity, and the relevance of Dectin-1 to this process, implies the existence of an invasin-independent mode of epithelial entry for A. fumigatus. In our studies cytochalasin D imposed an incomplete block upon spore internalisation suggesting that at least a subset of fungal elements can access the internal environment of epithelial cells via an ‘active penetration’ mechanism, as recently documented for C. albicans [65]. These important differences in the way in which different fungal pathogens interact with physiologically distinct epithelia highlight the current paucity of information on fungal interactions with pulmonary epithelia and, given that the vast majority of invasive mycoses are initiated via inhalation of fungal particles [1], should prompt renewed scrutiny of fungal interactions with mammalian lung tissues.

The mechanism by which epithelial cells recognise and internalise A. fumigatus conidia remains poorly characterised, as does the relevance of such activity to disease outcome. Our study demonstrates that uptake of A. fumigatus spores, by type II pneumocytes, is dependent upon a) actin polymerisation b) fungal cell wall/surface composition c) integrity of PacC and d) the β-1,3-glucan receptor Dectin-1, and moreover, that such interactions can negatively impact epithelial integrity. Dectin-1 expression in non-myeloid cells is increasingly frequently reported and has demonstrated relevance in β-1,3-glucan-(curdlan) exposed bronchiolar and alveolar type II cells [43], poly IC challenge of human bronchial epithelial cells [66], Mycobacterium ulcerans infection of epidermal keratinocytes and Mycobacterium tuberculosis infection of A549 epithelia [67], [68]. The A549 cell surface constitutively expresses Dectin-1, regardless of infection by A. fumigatus [44]. In humans, a Y238X Dectin-1 polymorphism is a risk factor for invasive aspergillosis in haematopoietic stem cell recipients. Cunha et al. (2010) found, in experimental HSCT, that transplant of stem cells from Dectin-1- donors to wild-type recipients resulted in lessened susceptibility to invasive aspergillosis. Thus by restricting the Dectin-1 deficiency to cells of myeloid origin, susceptibility to invasive aspergillosis was not altered. We found Dectin-1 deficiency, in the absence of leukocytes, to heighten epithelial damage in the whole animal host relative to leukopenic wild-type animals. This observation and several of our findings support a curative role for Dectin-1 mediated internalisation of A. fumigatus spores. According to Han et al., 2011, internalisation of A. fumigatus by A549 epithelial cells can be correlated with membrane phosphatidylcholine cleavage, a process which is closely linked to alteration of cytoskeletal actin dynamics, and prompted by exposure to β-1,3-glucan. This finding is consistent with our observation that cell wall extracts and killed A. fumigatus hyphae can perturb epithelial integrity. Our data, and those of Chaudhary et al., 2012, who found that bronchial ECs from cystic fibrosis sufferers demonstrate impaired uptake and killing of conidia, are highly suggestive of a curative role for EC activities during exposure to A. fumigatus spores. It does, however, remain feasible that the pulmonary epithelium provides a reservoir for A. fumigatus spores, and the attenuated phenotype of the ΔpacC mutant is consistent with such a theory. It also remains feasible that contact-dependent perturbation of epithelia facilitates subsequent protease-mediated damage by exposing subepithelial structures and facilitating fungal adhesion. Studies of C. albicans have revealed several means of fungal entry into epithelial cells, including self-induced endocytosis, and protease-mediated decay, the latter impacting, via Rim101-mediated E-cadherin degradation, the disintegration of oral epithelia [69]. It is most likely that multiple mechanisms contribute also to the pathogenicity of A. fumigatus. What is unique about PacC in A. fumigatus, is the critical role played by PacC-dependent factors in all of these processes and the profound requirement for PacC to orchestrate epithelial entry, protease-mediated epithelial decay, invasive growth and pathogenicity. These findings not only identify PacC as a critical master regulator of pathogenicity determinants in A. fumigatus, but also heighten its relevance as an antifungal target.

Materials and Methods

Fungal strains, media and treatments

A. fumigatus strains used in this study are listed in Table S1. A. fumigatus strains were cultured at 37°C in Aspergillus Minimal Media (AMM) or Aspergillus Complete Media (ACM) [70]. For preparation of A. fumigatus culture supernatants, 106 spores/ml were grown in Dulbecco's Modified Eagle Medium (DMEM, Sigma) supplemented with 10% foetal bovine serum (FBS, Sigma) and 10% penicillin and streptomycin (Sigma) at 37°C, 5% CO2 for either 16, 48, 60 or 72 hr. Supernatants were doubly filtrated through Miracloth and centrifuged for 10 min at 4000 rpm to remove any hyphal fragments. To inhibit protease activity in culture supernatants, filtrates were treated with the serine and cysteine protease inhibitor antipain (10 µg/ml) for 1 hr. For preparation of A. fumigatus cell wall extracts, see Text S1. For analyses of cell wall composition, A. fumigatus strains were harvested from an ACM plate (0 hr) as previously described or from 105 spores/ml cultures grown in AMM broth for 4, 8 and 16 hr at 37°C with shaking at 200 rpm. For in vitro challenge of epithelial monolayers with killed hyphae 104 spores/ml were incubated in supplemented DMEM at 37°C, 5% CO2 for 18 hr (parental isolates and reconstituted strains) or 36 hr (ΔpacC mutants). A. fumigatus hyphae were killed by incubating them in PBS supplemented with 0.02% thimerosal (Sigma) overnight at 4°C [71], a treatment which preserves cellular integrity. Before incubation with monolayers, killed hyphae were washed twice in PBS. Killing was verified by plating a 1∶100 dilution of killed hyphae in ACM plates.

Generation of ΔpacC mutants

ΔpacC mutants in the genetic backgrounds CEA10 (ΔpacCCEA10) and ATCC46645 (ΔpacCATCC) were constructed by gene replacement (Figure S1A) using a split-marker strategy [72]. For details, see Text S1. Initial phenotypic analyses, including survival analyses were performed using both ΔpacCATCC and ΔpacCCEA10 mutants, while subsequent analyses of gene expression were limited to the ΔpacCATCC mutant. For analyses of ΔpacC fungal burden in mice we opted to use the lesser attenuated ΔpacCCEA10 to prolong fungal occupancy of the murine lung.

Aspergillus phenotypic analysis

Dilutions of 103 conidia were inoculated onto ACM or supplemented AMM (as shown on Table S3) and incubated for 48 hr and 72 hr respectively. Images were captured using a Nikon Coolpix 990 digital camera.

Electromobility shift assays

Spores were inoculated at a density of 1×106 to 2×106 spores/ml, in 100 ml of liquid ACM, and grown for 16 hr at 37°C. Next, media was buffered to pH 5.0 with 100 mM glycolic acid pH 5.0 or to pH 8.0 with 100 mM Tris-HCl pH 8.0, pH shifts were performed for 1 hour. 10 mg of protein was extracted from washed mycelia as described previously [73]. Protein concentrations were determined using the Bradford assay [74]. The ipnA2 probe was synthesised and labelled as described previously [27], [73]. Densitometry data were obtained by measuring pixel intensity/mm2 for the relevant bands using a Phosphorimager FLA-3000 (FujiFilm) and Multi-Gauge V3.0 software.

Murine infections

Murine infections were performed under UK Home Office Project Licence PPL/70/6487 in dedicated facilities at Imperial College London. For all experiments A. fumigatus spores were harvested and prepared as previously described [75] and viable counts from administered inocula were determined, following serial dilution, by growth for 24–48 hr on ACM. Mice were housed in individually vented cages and anaesthetized by halothane inhalation and infected by intranasal instillation of spore suspensions. Mice were rendered leukopenic by administration of cyclophosphamide (150 mg/kg, intraperitoneal) on days −3, −1, +2 and every subsequent third day, and a single subcutaneous dose of hydrocortisone acetate (112.5 mg/kg) administered on day −1.

Survival analysis. Leukopenic male CD1 mice (18–22 g) were infected by intranasal instillation of 5.0 × 104 or 6.0 × 105 conidia in 40 µl of saline solution. Mice were weighed every 24 hr from day of infection and visual inspection made twice daily. In the majority of cases the end-point for survival experimentation was a 20% reduction in body weight measured from day of infection, at which point mice were sacrificed.

Histological and transcriptomic analyses. Leukopenic male CD1 mice (n  =  8) were infected with 108 conidia in 40 µl of saline solution. At the relevant time-points post-infection, mice were sacrificed and lungs were partitioned, using surgical sutures, into lobes destined for transcriptomic or histological analysis. Bronchoalveolar lavages (BALs) were performed using three 0.5 ml aliquots of pre-warmed sterile saline. BALs were snap frozen immediately following harvesting using liquid nitrogen. Lobes for histological sectioning were removed and immediately fixed in 4% (v/v) formaldehyde (Sigma). Lungs were embedded in paraffin prior to sectioning and stained with haematoxylin and eosin or light green and Grocott's Methenamine Silver. Images were taken using a Reichert-Jung (Slough, UK) Polyvar microscope using brightfield illumination at 40X magnification.

Fungal burden analyses. Immunosuppressed male CD1 mice (n  =  5) were infected with 3.75 × 105 spores. Mice were culled and whole lungs were collected after 24 and 48 hr of infection.

Antifungal drug susceptibility.

To test susceptibility to caspofungin, leukopenic, male CD1 mice (n  =  5) were infected with 3 × 104 spores in 40 µl of saline solution and treated with 5 mg/kg caspofungin by intraperitoneal injection on days −3, −1 and +1. Lungs were homogenised, serially diluted and cultured in duplicate in a serial dilution series of up to 10−4, on ACM.

Cellular content of BALs.

Immunocompetent male CD1 mice were infected with 106 spores in 40 µl of saline solution. Mice were culled after 24 hr and BALs were collected using three 0.5 ml aliquots of sterile saline.

Assessment of epithelial damage.

Leukopenic male CD1 and C57BL/6 Dectin-1−/− [76] were infected with 106 spores in 40 µl of saline solution and culled after 24 hr of infection. Lungs were collected for histopathology and western blotting. BALs, collected using three 0.5 ml aliquots of pre-warmed sterile saline, were used for LDH quantification.

Temporal analyses of A. fumigatus gene expression during murine infection

BAL samples were centrifuged at 14000 rpm for 5 min and the pellet was washed with 500 µl ice cold H2O to lyse host cells. Seven BALs were pooled, resuspended in 450 µl ME-RLC buffer (QIAGEN) and ground in liquid nitrogen with a pestle and mortar. RNA was then extracted using RNeasy Kit (QIAGEN). A reference RNA sample was extracted from A. fumigatus ATCC46645 conidia harvested from an ACM plate. Conidia were washed thoroughly with sterile water, quickly frozen in liquid nitrogen, and disrupted by grinding. Total RNA was extracted using RNeasy Kit (QIAGEN). The quality of RNA used for microarray analysis was checked using a Nanodrop ND-1000 Spectrophotometer (Nanodrop, Wilmington, USA). Only RNA with an A260/280 and an A260/230 ratio> 1.9 was used for the experiments. Labelled cDNA samples were synthesised as described previously [30]. Protocols for direct labelling and hybridisation of cDNA probes can be found on the JCVI website ( The A. fumigatus oligonucleotide slides version 3 was used for microarray hybridization ( phase- or strain-specific comparative analysis of gene expression datasets was conducted in Genespring GX 11.02 (Agilent). Normalised log2 expression ratios were filtered on expression level and differentially regulated transcripts were defined as having log2 (Cy5/Cy3) greater than the arbitrary thresholds of ± 1.5. Raw data have been deposited in the Gene Expression Omnibus (GEO) ( under accession number GSE54810. Functional analysis of differentially-expressed gene cohorts was implemented by DAVID ( [77], [78]. Microarray data was validated by qPCR as described in Text S1.

Analysis of A549 epithelial monolayer integrity

Human pulmonary carcinoma epithelial cell line A549 (American type culture collection, CCL-185) was used throughout this study. For all experiments, cells were maintained at 37°C, 5% CO2 in supplemented DMEM. Epithelial cells were used after the second or third passage. For all experiments, 105 A549 cells were seeded in 6-well tissue culture plates and incubated to ≥ 90% confluence. Monolayers were challenged with 105 spores/ml, 200 µl of supernatant or 200 µl of cell wall extract. Following co-incubation with A. fumigatus spores, cell wall extracts or supernatants, monolayers were washed 3 times with PBS and adherent A549 cells were counted in 3 fields of view at magnifications of 20 or 40 (Nikon Eclipse TS100). Washing was omitted for analyses of contact-dependent damage.

51chromium release assay

Damage to A549 epithelial cells by the various strains of A. fumigatus was determined using a previously described method at 16, 20 and 24 hr of co-incubation [35]. The 51Cr content of the medium and lysates was measured and the degree of epithelial cell damage was calculated and corrected for spontaneous chromium release by uninfected epithelial cells.

A. fumigatus cell wall analysis

Live-cell microscopy.

Fungal cell walls were visualized using the chitin binding dye calcofluor white (Sigma). 105 conidia were grown in 8-well slide culture chambers in AMM (pH 6.5) at 28°C for 17–18 hr and stained with 10 µg/ml of calcofluor white for 5 min prior imaging on a Nikon Eclipse TE2000E microscope with DIC optics, a 60× (1.3 NA) plan fluor objective, and equipped with an ORCA-ER CCD camera (Hamamatsu, Welwyn Garden City, UK) driven by the MetaMorph NX1.1 software for image acquisition. For calcofluor white, a Nikon UV-2A filter cube (excitation filter 355/15 nm BP, dichroic mirror 400 nm LP, emission filter 420 nm LP) was used. Images were processed and analysed using the software Image J version 1.47. Images show maximum intensity projections with inverted look-up tables (LUTs).

Electron microscopy.

Preparation of samples for Transmission Electron Microscopy (TEM) were performed as previously described [79]. See Text S1.

Preparation of cell wall extracts for challenge of monolayer integrity and composition analysis.

Cell walls were extracted with some modifications as described previously [80], [81]. See Text S1.


To analyse the localisation of α-1,3-glucan or β-1,3-glucan on A. fumigatus cell walls, isolates (105 or 104 spores/ml) were grown in 8-well slide culture chambers (Nalge Nunc International, Rochester, NY) in supplemented DMEM for 4, 8, 12 or 16 hr. α-1,3-glucan was visualized using 0.1 mg/ml mouse IgMγ MOPC-104E (Sigma, in PBS buffer) as primary antibody and 0.1 mg/ml Alexa Fluor 488 goat anti-mouse IgM (μ chain) antibody (Life technologies, in PBS buffer) [47], [82], [83]. β-1,3-glucan was visualized 5 µg/ml Fc-dectin-1 fusion (kind gift from Dr G.D. Brown, University of Aberdeen) coupled with 15 µg/ml goat anti-human IgG (H+L) Fluorescein conjugated antibody [45], [46]. Briefly, samples were incubated with primary antibodies for 30 minutes, before incubation with the secondary antibodies for 30 minutes in the dark.

To visualise epithelial monolayers co-incubated with A. fumigatus strains, A549 cells were seeded in 2-well slide culture chambers (Nalge Nunc International, Rochester, NY) in supplemented DMEM. At 90% confluence, epithelial monolayers were incubated with A. fumigatus isolates (105 spores/ml) for 16 hr. After washing the monolayers three times with PBS, samples were incubated in supplemented DMEM with 10 µg/ml FITC-labelled concanavalin A (Molecular Probes) and 0.4 mg/ml calcofluor white (Sigma), to visualize respectively epithelial cells and hyphae. Labelling was performed for 30 minutes at 37°C, 5% CO2.

After rinsing with PBS, samples were imaged using a Nikon Eclipse TE2000E microscope with DIC optics, a 20× plan fluor objective or 60× (1.3 NA) plan fluor objective, and equipped with an ORCA-ER CCD camera (Hamamatsu, Welwyn Garden City, UK) driven by the MetaMorph NX1.1 software for image acquisition. For Alexa Fluor 488, FITC and fluorescein, a Nikon B-2A filter cube (excitation filter 470/20 nm BP, dichroic mirror 500 nm LP, emission filter 515 nm LP) was used. For calcofluor white, a Nikon UV-2A filter cube (excitation filter 355/15 nm BP, dichroic mirror 400 nm LP, emission filter 420 nm LP) was used. Images were processed and analysed using the software Image J version 1.47.

Adhesion assay

Adhesion was tested using a modification of the protocol in Gravelat et al., 2012 [84] as described in Text S1.

Internalisation of A. fumigatus spores by A549 epithelia

Pretreatment of epithelia.

For evaluation of detachment or nystatin protection assay, epithelial monolayers were pre-treated for 1 hour with 0.2 µM cytochalasin D (CD, Sigma, resuspended in DMSO) or 0.3 µg/ml α-Dectin-1 antibody (R & D) or 0.3 µg/ml Mouse IgG2B Isotype Control (Clone 20116) (R & D).

Nystatin protection assay.

A549 density was checked by enumeration, and epithelial monolayers were infected with 106 spores/ml. Viable counts of inocula were determined following serial dilution by plating on ACM and growth for 24–48 hr. The nystatin protection assay was performed as in Wasylnka et al., 2002 [18] allowing spore internalisation for 4 hr. The percentage of internalisation was calculated relative to the total amount of conidia inoculated and applying a correction for an MOI of 1. Experiments were performed in technical and biological duplicate for wild-types and triplicate for ΔpacC mutants. Susceptibility of the strains to nystatin was verified as described in Text S1.

LDH assay

The release of lactate dehydrogenase (LDH) was assessed in BALs using the Cytox 96 Non-Radioactive Cytotoxicity Assay kit (Promega) according to manufacturer's instructions. BAL samples were assessed in triplicate and averaged values were normalised to the total amount of protein as measured in triplicate using a bicinchoninic acid assay (BCA) assay (Sigma) according to manufacturer's instructions.

Western blotting

Lungs were homogenised in 1 ml of PBS (pH 7.4) containing protease inhibitor cocktail (Roche) and protein concentration was measured by BCA, using a BSA as standard (Sigma). 9 µg of protein was analysed by western blotting [85]. A 1∶1000 dilution of a α-S100B antibody (Abcam) was used, in parallel with an α-actin antibody (Cell Signaling) for normalisation of loading.

FACS analysis of BALs

BALs were collected using 3 ml of PBS and a further 5 ml of PBS were added at the time of preparation of the samples for FACS analysis. Cell pellets were resuspended in 1 ml red blood lysis buffer (Sigma). Blocking of the Fc receptor to remove unspecific signal was achieved by incubating the samples with 0.5 µg of an anti-Mouse CD16/CD32 antibody (E-bioscience) in 100 µl of 0.1% BSA PBS. 14 µl of antibody mix was added for labelling of macrophages (α-F4/80-APC-Cy7, 5 µl, Biolegend), leukocytes (α-CD45-PE, 2 µl, E-bioscience) and neutrophils (α-Ly-6G-BV421, 2 µl, Biolegend). Samples was analysed using a BD Fortessa cell analyser. Data acquisition and analysis were performed using respectively the software Diva and FlowJo. For each sample (n  =  4, plus 2 controls), cell population size for macrophages (F4/80+) and neutrophils (Ly-6G+) were expressed as cells/ml.

Antifungal susceptibility

In vitro susceptibility testing of A. fumigatus strains was performed according to the European Committee for Antimicrobial Susceptibility testing (EUCAST) standard method [53]. Caspofungin was tested on A. fumigatus strains in biological and technical triplicate. 1.25 × 105 strains were grown with RPMI1640, 0.165 mol/L MOPS, pH 7.0 and incubated at 37°C for 48 hr. The final concentration of caspofungin tested ranged from 0.03 to 16 ug/ml.

Statistical analysis of data

GraphPad Prism was used to interpret data and p values were calculated through Log Rank analysis (for comparative survival), unpaired t tests or 1-way ANOVA tests as indicated. Error bars show the Standard Error of the Mean (SEM). ***p<0.001, 0.001 <**p<0.01, and 0.01 <*p<0.05

Online supporting information

Figure S1 shows the strategies for construction and validation of A. fumigatus ΔpacC mutants. Figure S2 shows growth of A. fumigatus isolates on laboratory culture media, as images and as radial growth rates normalised to pH 6.5. Figure S3 shows pH-dependency of PacC processing, as measured using EMSA analyses. Figure S4 shows the experimental set-up and outputs of in-host transcriptomic analysis of A. fumigatus wild-type and ΔpacC activities. Figure S5 shows a heat map of differentially expressed A. fumigatus gene products having predicted signal peptides. Figure S6 shows a heat map of differentially expressed A. fumigatus gene products having putative or demonstrated roles in cell wall biosynthesis. Fig. S7 shows a heat map of differentially expressed A. fumigatus gene products involved in gliotoxin biosynthesis (AFUA_6G09570-AFUA_6G09740). Figure S8 shows qPCR validation of microarray data. Figure S9 shows analysis of A. fumigatus protease activity using a qualitative gelatine degradation assay. Figure S10 shows the electron microscopy of A. fumigatus ΔpacCATCC mutant and the respective parental isolate at 0, 4, 8 and 16 hr of growth. Figure S11 shows equivalent nystatin-mediated killing of wild type and mutant isolates used in this study. Figure S12 shows equivalent adhesion of mutant and wild types isolates to plastic, and to epithelia in vitro. Figure S13 shows immunofluorescence analysis of α-glucan distribution in A. fumigatus germlings. Table S1 and S2 list the A. fumigatus strains and oligonucleotides used in this study respectively. Table S3 lists the A. fumigatus phenotypic testing conditions tested. Dataset S1 shows the temporal analysis of A. fumigatus gene expression during intiation of murine pulmonary aspergillosis. Dataset S2 shows the genes differentially regulated, relative to wild type, in a host-infecting A. fumigatus ΔpacCATCC mutant. Dataset S3 shows the expression of genes encoding secreted gene products which are regulated by either PrtT [9] or PacC, or both transcription factors. Text S1 contains the supplementary material and methods.

Accession numbers

The genes and gene products (with accession numbers at studied in this work is pacC (AFUA_3G11970). Also mentioned in the text are prtT (AFUA_4G10120), mep (AFUA_8G07080), alp1 (AFUA_4G11800), β-tubulin (AFUA_7G00250) and the gliotoxin cluster (AFUA_6G09570-AFUA_6G09740).

Supporting Information

Dataset S1.

Temporal analysis of A. fumigatus gene expression during initiation of murine pulmonary aspergillosis. Differentially-expressed genes (log2 ratios ≥ +/− 1.5 relative to ungerminated spores) were categorised as INVARIANT UP/DOWN (differentially expressed at all time points of analysis), EARLY UP/DOWN (differentially expressed at any or all of 4, 8 and 12 hours post-infection) and LATE UP/DOWN (differentially expressed at either or both of 12 and 16 hours post-infection). Functional analysis of differentially-expressed gene cohorts was implemented by DAVID (


Dataset S2.

Genes differentially regulated, relative to wild type, in a host-infecting A. fumigatus ΔpacCATCC mutant. Differentially-expressed genes (log2 ratios ≥ +/− 1.5 relative to wild type) were categorised as ALWAYS UP/DOWN or UP/DOWN at ≥ one time point of infection. Functional analysis of differentially-expressed gene cohorts was implemented by DAVID (


Dataset S3.

Expression of genes encoding secreted gene products which are regulated by either PrtT or PacC, or both transcription factors.


Figure S1.

Construction and validation of A. fumigatus ΔpacC mutants. Schematic for the construction of A. fumigatus ΔpacC mutants by gene replacement using a split pyrithiamine resistance marker (A) and Southern blot analysis of A. fumigatus wild-type and ΔpacC mutants (B). According to the first strategy employed, genomic DNA on indicated strains was digested with SalI and probed with two hybridisation probes generated using the oligonucleotides PacCSB1 & PacCSB2 (Probe 1) and LucPtrAF & LucPtrAR (Probe 3) (Table S2). The expected signals for Probe 1 were 7883 bp for the wild-type and 3355 bp for the ΔpacC mutants. For Probe 3, no signal was expected for the wild-type, whereas for a single, homologous integration of the deletion cassette the expected signal was 3355 bp. According to the second strategy employed, genomic DNA of indicated strains was digested with EcoRV and probed with a hybridisation probe generated using oligonucleotides opacC3 and opacC6 (Probe 2) (Table S2). The expected signals for Probe 3 were 3709 bp for the wild-type and 3501 bp for the ΔpacC mutants.


Figure S2.

Colonial growth of wild type and ΔpacC mutants. (A) Colonial growth phenotypes on ACM, 48 hr of growth, 103 conidia. (B) Percent radial growth at pH 8.0 relative to pH 6.5, 72 hr of growth, 103 conidia, n  =  3, unpaired t test, *** p<0.001 and ** 0.001 <p<0.01. (C) Percent radial growth at pH 7.2 relative to pH 6.5, 72 hr of growth, 103 conidia, n  =  3.


Figure S3.

Processing of A. fumigatus PacC. (A) PacC processing after shift to acidic (pH 5.0) and alkaline (pH 8.0) by EMSA. Low mobility and high mobility forms of PacC are indicated on the right side. (B) Densitometry plot of EMSA data expressed, per complex, as a function of total PacC protein.


Figure S4.

In-host transcriptomic analysis of A. fumigatus wild-type and ΔpacC activities. (A) Experimental design depicting hybridisation schemes. (I) Analysis of wild-type temporal transcription profile during initiation of murine infection comparing gene expression at 4 independent time points (4, 8, 12 and 16 hr) to a common RNA reference extracted from wild-type spores. (II) Analysis of ΔpacC temporal transcription profile during initiation of murine infection comparing gene expression at 4 independent time points (4, 8, 12 and 16 hr) to a common RNA reference extracted from ΔpacC spores. (III) Comparative, stage-specific, analysis of ΔpacC and wild-type transcript profiles during initiation of murine infection (4, 8, 12 and 16 hr). (B, C, D) Up- and down-regulated genes (cut-off ± 1.5) for the wild-type (B), ΔpacC (C) and comparative (D) time courses. Venn diagrams depict the numbers of genes differentially regulated at each time point of the analyses. Profile plots indicate temporal behaviours of all differentially regulated genes relative to the 4 hr time point.


Figure S5.

Heat-map depiction of temporal in-host gene expression for wild type and ΔpacC. Heat maps depict results from time-series infection studies and profile gene expression for predicted secreted proteins. Colouration indicates magnitude of log2 ratio relative to RNA reference (ungerminated spores).


Figure S6.

Heat-map depiction of temporal in-host gene expression for wild type and ΔpacC. Heat maps depict results from time-series infection studies and profile gene expression for predicted cell wall biosynthetic gene products. Colouration indicates magnitude of log2 ratio relative to RNA reference (ungerminated spores).


Figure S7.

Heat-map depiction of temporal in-host gene expression for wild type and ΔpacC. Heat maps depict results from time-series infection studies and profile gene expression for genes (AFUA_6G09570-AFUA_6G09740; AFUA_6G09745 omitted from the microarray) of the gliotoxin cluster. Colouration indicates magnitude of log2 ratio relative to RNA reference (ungerminated spores).


Figure S8.

qPCR validation of microarray data. Accuracy of microarray data was independently verified by quantitative RT-PCR on selected transcripts, values (A) and graphical representation (B). Oligonucleotides used for this analysis are detailed in Table S2. Fold change due to treatment (-1/ΔCT) was calculated using A. fumigatus Act1 (AFUA_6G04740) as a house-keeping gene.


Figure S9.

Qualitative analysis of A. fumigatus protease activity in cell culture filtrates. Culture supernatant (50 µl of supplemented DMEM + A549 cell culture, 106 spores/ml) was spotted onto X-ray film, incubated at 42°C and washed after overnight digestion with water. Positive control is represented by trypsin (50 BAEE units). Trypsin hydrolyzes N-benzoyl-L-arginine ethyl ester (BAEE) and one BAEE unit equals the amount of the enzyme determining an increase in absorbance of 0.001 per minute at 25°C and 253 nm.


Figure S10.

Electron microscopy of A. fumigatus ΔpacCATCC mutant and the respective parental isolate at 0, 4, 8 and 16 hr of growth.


Figure S11.

Nystatin-mediated killing of wild type and ΔpacC mutant spores.


Figure S12.

Adhesion of wild type and ΔpacC mutant spores to plastic and A549 monolayers.


Figure S13.

Immunofluorescence-mediated imaging of A. fumigatus α-glucan.


Table S1.

A. fumigatus strains used in this study.


Table S2.

Oligonucleotides used in this study.


Table S3.

A. fumigatus phenotypic testing.


Text S1.

Supplementary material and methods.



We would like to thank Prof. Y. Iwakura (Tokyo University of Science, Japan) for kindly providing us with the Dectin-1−/− mice. Fc-dectin-1 fusion construct for immunofluorescence and analysis of surface exposed β-glucans was a generous gift from Prof. G.D. Brown, (University of Aberdeen, UK). We also thank Dr. B Frank (JCVI, USA) for technical assistance with quantitative PCR analyses.

Author Contributions

Conceived and designed the experiments: MB MS LAF TCC AM LAW SH MS AMC DC HL SS NDF DAJ CAM NDR SGF EAE WCN HH EMB. Performed the experiments: MB MS LAF TCC AM LAW SH MS AMC DC HL SS NDF EAE EMB. Analyzed the data: MB MS LAF TCC AM LAW SH MS AMC DC HL SS NDF DAJ CAM NDR SGF EAE WCN HH EMB. Contributed reagents/materials/analysis tools: SS DAJ CAM NDR SGF EAE WCN HH EMB. Wrote the paper: MB EMB. Critically revised the manuscript: MB MS LAF TCC AM LAW SH MS AMC DC HL SS NDF DAJ CAM NDR SGF EAE WCN HH EMB.


  1. 1. Brown GD, Denning DW, Gow NA, Levitz SM, Netea MG, et al. (2012) Hidden killers: human fungal infections. Sci Transl Med 4 165: 165rv13.
  2. 2. Baddley JW, Andes DR, Marr KA, Kontoyiannis DP, Alexander BD, et al. (2010) Factors associated with mortality in transplant patients with invasive aspergillosis. Clin Infect Dis 50 12: 1559–67.
  3. 3. Kontoyiannis DP, Marr KA, Park BJ, Alexander BD, Anaissie EJ, et al. (2010) Prospective surveillance for invasive fungal infections in hematopoietic stem cell transplant recipients, 2001-2006: overview of the Transplant-Associated Infection Surveillance Network (TRANSNET) Database. Clin Infect Dis 50 8: 1091–100.
  4. 4. Pappas PG, Alexander BD, Andes DR, Hadley S, Kauffman CA, et al. (2010) Invasive fungal infections among organ transplant recipients: results of the Transplant-Associated Infection Surveillance Network (TRANSNET). Clin Infect Dis 50 8: 1101–11.
  5. 5. Denning DW, Pleuvry A, Cole DC (2011) Global burden of chronic pulmonary aspergillosis as a sequel to pulmonary tuberculosis. Bull World Health Organ 89 12: 864–72.
  6. 6. Morgan J, Wannemuehler KA, Marr KA, Hadley S, Kontoyiannis DP, et al. (2005) Incidence of invasive aspergillosis following hematopoietic stem cell and solid organ transplantation: interim results of a prospective multicenter surveillance program. Med Mycol 43 Suppl 1 S49–58.
  7. 7. Amitani R, Taylor G, Elezis EN, Llewellyn-Jones C, Mitchell J, et al. (1995) Purification and characterization of factors produced by Aspergillus fumigatus which affect human ciliated respiratory epithelium. Infect Immun 63 9: 3266–71.
  8. 8. Kogan TV, Jadoun J, Mittelman L, Hirschberg K, Osherov N (2004) Involvement of secreted Aspergillus fumigatus proteases in disruption of the actin fiber cytoskeleton and loss of focal adhesion sites in infected A549 lung pneumocytes. J Infect Dis 189 11: 1965–73.
  9. 9. Sharon H, Hagag S, Osherov N (2009) Transcription factor PrtT controls expression of multiple secreted proteases in the human pathogenic mold Aspergillus fumigatus. Infect Immun 77 9: 4051–60.
  10. 10. Bergmann A, Hartmann T, Cairns T, Bignell EM, Krappmann S (2009) A regulator of Aspergillus fumigatus extracellular proteolytic activity is dispensable for virulence. Infect Immun 77 9: 4041–50.
  11. 11. Hartmann T, Cairns TC, Olbermann P, Morschhauser J, Bignell EM, et al. (2011) Oligopeptide transport and regulation of extracellular proteolysis are required for growth of Aspergillus fumigatus on complex substrates but not for virulence. Mol Microbiol 82 4: 917–35.
  12. 12. Ibrahim-Granet O, D'Enfert C (1997) The Aspergillus fumigatus mepB gene encodes an 82 kDa intracellular metalloproteinase structurally related to mammalian thimet oligopeptidases. Microbiology 143 (Pt 7) 2247–53.
  13. 13. Jaton-Ogay K, Paris S, Huerre M, Quadroni M, Falchetto R, et al. (1994) Cloning and disruption of the gene encoding an extracellular metalloprotease of Aspergillus fumigatus. Mol Microbiol 14 5: 917–28.
  14. 14. Reichard U, Monod M, Odds F, Ruchel R (1997) Virulence of an aspergillopepsin-deficient mutant of Aspergillus fumigatus and evidence for another aspartic proteinase linked to the fungal cell wall. J Med Vet Mycol 35 3: 189–96.
  15. 15. Tang CM, Cohen J, Krausz T, Van Noorden S, Holden DW (1993) The alkaline protease of Aspergillus fumigatus is not a virulence determinant in two murine models of invasive pulmonary aspergillosis. Infect Immun 61 5: 1650–6.
  16. 16. DeHart DJ, Agwu DE, Julian NC, Washburn RG (1997) Binding and germination of Aspergillus fumigatus conidia on cultured A549 pneumocytes. J Infect Dis 175 1: 146–50.
  17. 17. Paris S, Boisvieux-Ulrich E, Crestani B, Houcine O, Taramelli D, et al. (1997) Internalization of Aspergillus fumigatus conidia by epithelial and endothelial cells. Infect Immun 65 4: 1510–4.
  18. 18. Wasylnka JA, Moore MM (2002) Uptake of Aspergillus fumigatus conidia by phagocytic and nonphagocytic cells in vitro: quantitation using strains expressing green fluorescent protein. Infect Immun 70 6: 3156–63.
  19. 19. Gomez P, Hackett TL, Moore MM, Knight DA, Tebbutt SJ (2010) Functional genomics of human bronchial epithelial cells directly interacting with conidia of Aspergillus fumigatus. BMC Genomics 11 358.
  20. 20. Wasylnka JA, Moore MM (2003) Aspergillus fumigatus conidia survive and germinate in acidic organelles of A549 epithelial cells. J Cell Sci 116 Pt 8: 1579–87.
  21. 21. Osherov N (2012) Interaction of the pathogenic mold Aspergillus fumigatus with lung epithelial cells. Front Microbiol 3 346.
  22. 22. Chaudhary N, Datta K, Askin FB, Staab JF, Marr KA (2012) Cystic fibrosis transmembrane conductance regulator regulates epithelial cell response to Aspergillus and resultant pulmonary inflammation. Am J Respir Crit Care Med 185 3: 301–10.
  23. 23. Caddick MX, Brownlee AG, Arst HN Jr (1986) Regulation of gene expression by pH of the growth medium in Aspergillus nidulans. Mol Gen Genet 203 2: 346–53.
  24. 24. Davis D, Wilson RB, Mitchell AP (2000) RIM101-dependent and-independent pathways govern pH responses in Candida albicans. Mol Cell Biol 20 3: 971–8.
  25. 25. Davis D, Edwards JE Jr, Mitchell AP, Ibrahim AS (2000) Candida albicans RIM101 pH response pathway is required for host-pathogen interactions. Infect Immun 68 10: 5953–9.
  26. 26. Li W, Mitchell A (1997) Proteolytic activation of Rim1p, a positive regulator of yeast sporulation and invasive growth. Genetics 145 1: 63.
  27. 27. Tilburn J, Sarkar S, Widdick DA, Espeso EA, Orejas M, et al. (1995) The Aspergillus PacC zinc finger transcription factor mediates regulation of both acid- and alkaline-expressed genes by ambient pH. EMBO J 14 4: 779–90.
  28. 28. Davis D (2003) Adaptation to environmental pH in Candida albicans and its relation to pathogenesis. Current genetics 44 1: 1–7.
  29. 29. Bignell E, Negrete-Urtasun S, Calcagno A, Haynes K, Arst H Jr, et al. (2005) The Aspergillus pH-responsive transcription factor PacC regulates virulence. Molecular microbiology 55 4: 1072–1084.
  30. 30. McDonagh A, Fedorova ND, Crabtree J, Yu Y, Kim S, et al. (2008) Sub-Telomere Directed Gene Expression during Initiation of Invasive Aspergillosis. PLoS Pathog 4 9: e1000154.
  31. 31. Peñalva M, Tilburn J, Bignell E, Arst H Jr (2008) Ambient pH gene regulation in fungi: making connections. Trends in microbiology 16 6: 291–300.
  32. 32. Grahl N, Puttikamonkul S, Macdonald JM, Gamcsik MP, Ngo LY, et al. (2011) In vivo hypoxia and a fungal alcohol dehydrogenase influence the pathogenesis of invasive pulmonary aspergillosis. PLoS Pathog 7 7: e1002145.
  33. 33. Amich J, Vicentefranqueira R, Mellado E, Ruiz-Carmuega A, Leal F, et al. (2014) The ZrfC alkaline zinc transporter is required for Aspergillus fumigatus virulence and its growth in the presence of the Zn/Mn-chelating protein calprotectin. Cell Microbiol 16 4: 548–64.
  34. 34. Lewis RE, Wiederhold NP (2005) Murine model of invasive aspergillosis. Methods Mol Med 118 129–42.
  35. 35. Bezerra LML, Filler SG (2004) Interactions of Aspergillus fumigatus with endothelial cells: internalization, injury, and stimulation of tissue factor activity. Blood 103 6: 2143–2149.
  36. 36. Mellado E, Aufauvre-Brown A, Gow NA, Holden DW (1996) The Aspergillus fumigatus chsC and chsG genes encode class III chitin synthases with different functions. Mol Microbiol 20 3: 667–79.
  37. 37. Valiante V, Heinekamp T, Jain R, Hartl A, Brakhage AA (2008) The mitogen-activated protein kinase MpkA of Aspergillus fumigatus regulates cell wall signaling and oxidative stress response. Fungal Genet Biol 45 5: 618–27.
  38. 38. Dichtl K, Helmschrott C, Dirr F, Wagener J (2012) Deciphering cell wall integrity signalling in Aspergillus fumigatus: identification and functional characterization of cell wall stress sensors and relevant Rho GTPases. Mol Microbiol 83 3: 506–19.
  39. 39. Cheung AL, Ying P, Fischetti VA (1991) A method to detect proteinase activity using unprocessed X-ray films. Anal Biochem 193 1: 20–3.
  40. 40. Brown GD, Taylor PR, Reid DM, Willment JA, Williams DL, et al. (2002) Dectin-1 is a major β-glucan receptor on macrophages. J Exp Med 196 3: 407–12.
  41. 41. Brown GD, Herre J, Williams DL, Willment JA, Marshall AS, et al. (2003) Dectin-1 mediates the biological effects of β-glucans. J Exp Med 197 9: 1119–24.
  42. 42. Brown GD, Gordon S (2001) Immune recognition. A new receptor for beta-glucans. Nature 413 6851: 36–7.
  43. 43. Rand TG, Sun M, Gilyan A, Downey J, Miller JD (2010) Dectin-1 and inflammation-associated gene transcription and expression in mouse lungs by a toxic (1,3)-β-D glucan. Arch Toxicol 84 3: 205–20.
  44. 44. Han X, Yu R, Zhen D, Tao S, Schmidt M, et al. (2011) beta-1,3-Glucan-induced host phospholipase D activation is involved in Aspergillus fumigatus internalization into type II human pneumocyte A549 cells. PLoS One 6 7: e21468.
  45. 45. Graham LM, Tsoni SV, Willment JA, Williams DL, Taylor PR, et al. (2006) Soluble Dectin-1 as a tool to detect β-glucans. J Immunol Methods 314 1–2: 164–9.
  46. 46. Sousa Mda G, Reid DM, Schweighoffer E, Tybulewicz V, Ruland J, et al. (2011) Restoration of pattern recognition receptor costimulation to treat chromoblastomycosis, a chronic fungal infection of the skin. Cell Host Microbe 9 5: 436–43.
  47. 47. Rappleye CA, Eissenberg LG, Goldman WE (2007) Histoplasma capsulatum α-(1,3)-glucan blocks innate immune recognition by the β-glucan receptor. Proc Natl Acad Sci U S A 104 4: 1366–70.
  48. 48. Sorci G, Giovannini G, Riuzzi F, Bonifazi P, Zelante T, et al. (2011) The danger signal S100B integrates pathogen- and danger-sensing pathways to restrain inflammation. PLoS Pathog 7 3: e1001315.
  49. 49. Nobile CJ, Solis N, Myers CL, Fay AJ, Deneault JS, et al. (2008) Candida albicans transcription factor Rim101 mediates pathogenic interactions through cell wall functions. Cell Microbiol 10 11: 2180–96.
  50. 50. O'Meara TR, Norton D, Price MS, Hay C, Clements MF, et al. (2010) Interaction of Cryptococcus neoformans Rim101 and protein kinase A regulates capsule. PLoS Pathog 6 2: e1000776.
  51. 51. O'Meara TR, Holmer SM, Selvig K, Dietrich F, Alspaugh JA (2013) Cryptococcus neoformans Rim101 is associated with cell wall remodeling and evasion of the host immune responses. MBio 4 1.
  52. 52. O'Meara TR, Xu W, Selvig KM, O'Meara MJ, Mitchell AP, et al. (2014) The Cryptococcus neoformans Rim101 Transcription Factor Directly Regulates Genes Required for Adaptation to the Host. Molecular and Cellular Biology 34 4: 673–684.
  53. 53. EUCAST (2008) Subcommittee on Antifungal Susceptibility Testing (AFST) of the ESCMID European Committee for Antimicrobial Susceptibility Testing (EUCAST), EUCAST Technical Note on the method for the determination of broth dilution minimum inhibitory concentrations of antifungal agents for conidia-forming moulds. Clin Microbiol Infect 14 10: 982–4.
  54. 54. Eisendle M, Oberegger H, Buttinger R, Illmer P, Haas H (2004) Biosynthesis and uptake of siderophores is controlled by the PacC-mediated ambient-pH regulatory system in Aspergillus nidulans. Eukaryotic cell 3 2: 561.
  55. 55. Nierman WC, Pain A, Anderson MJ, Wortman JR, Kim HS, et al. (2005) Genomic sequence of the pathogenic and allergenic filamentous fungus Aspergillus fumigatus. Nature 438 7071: 1151–6.
  56. 56. Latge JP (1999) Aspergillus fumigatus and aspergillosis. Clin Microbiol Rev 12 2: 310–50.
  57. 57. Dagenais TR, Keller NP (2009) Pathogenesis of Aspergillus fumigatus in Invasive Aspergillosis. Clin Microbiol Rev 22 3: 447–65.
  58. 58. Kolattukudy PE, Lee JD, Rogers LM, Zimmerman P, Ceselski S, et al. (1993) Evidence for possible involvement of an elastolytic serine protease in aspergillosis. Infect Immun 61 6: 2357–68.
  59. 59. Markaryan A, Morozova I, Yu H, Kolattukudy PE (1994) Purification and characterization of an elastinolytic metalloprotease from Aspergillus fumigatus and immunoelectron microscopic evidence of secretion of this enzyme by the fungus invading the murine lung. Infect Immun 62 6: 2149–57.
  60. 60. Sharon H, Amar D, Levdansky E, Mircus G, Shadkchan Y, et al. (2011) PrtT-regulated proteins secreted by Aspergillus fumigatus activate MAPK signaling in exposed A549 lung cells leading to necrotic cell death. PLoS One 6 3: e17509.
  61. 61. Monod M, Paris S, Sarfati J, Jaton-Ogay K, Ave P, et al. (1993) Virulence of alkaline protease-deficient mutants of Aspergillus fumigatus. FEMS Microbiol Lett 106 1: 39–46.
  62. 62. Park H, Myers CL, Sheppard DC, Phan QT, Sanchez AA, et al. (2005) Role of the fungal Ras-protein kinase A pathway in governing epithelial cell interactions during oropharyngeal candidiasis. Cell Microbiol 7 4: 499–510.
  63. 63. Phan QT, Myers CL, Fu Y, Sheppard DC, Yeaman MR, et al. (2007) Als3 is a Candida albicans invasin that binds to cadherins and induces endocytosis by host cells. PLoS Biol 5 3: e64.
  64. 64. Sun JN, Solis NV, Phan QT, Bajwa JS, Kashleva H, et al. (2010) Host cell invasion and virulence mediated by Candida albicans Ssa1. PLoS Pathog 6 11: e1001181.
  65. 65. Wächtler B, Citiulo F, Jablonowski N, Förster S, Dalle F, et al. (2012) Candida albicans-Epithelial Interactions: Dissecting the Roles of Active Penetration, Induced Endocytosis and Host Factors on the Infection Process. PLoS One 7 5: e36952.
  66. 66. Melkamu T, Squillace D, Kita H, O'Grady SM (2009) Regulation of TLR2 expression and function in human airway epithelial cells. J Membr Biol 229 2: 101–13.
  67. 67. Lee HM, Yuk JM, Shin DM, Jo EK (2009) Dectin-1 is inducible and plays an essential role for mycobacteria-induced innate immune responses in airway epithelial cells. J Clin Immunol 29 6: 795–805.
  68. 68. Lee HM, Shin DM, Choi DK, Lee ZW, Kim KH, et al. (2009) Innate immune responses to Mycobacterium ulcerans via toll-like receptors and dectin-1 in human keratinocytes. Cell Microbiol 11 4: 678–92.
  69. 69. Villar CC, Kashleva H, Nobile CJ, Mitchell AP, Dongari-Bagtzoglou A (2007) Mucosal tissue invasion by Candida albicans is associated with E-cadherin degradation, mediated by transcription factor Rim101p and protease Sap5p. Infect Immun 75 5: 2126–35.
  70. 70. Pontecorvo G, Roper JA, Hemmons LM, Macdonald KD, Bufton AW (1953) The genetics of Aspergillus nidulans. Adv Genet 5 141–238.
  71. 71. Deighton FJ, Hall NK, Larsh HW (1979) Merthiolate treatment of pathogenic fungi. J Clin Microbiol 10 2: 144–6.
  72. 72. Nielsen ML, Albertsen L, Lettier G, Nielsen JB, Mortensen UH (2006) Efficient PCR-based gene targeting with a recyclable marker for Aspergillus nidulans. Fungal Genet Biol 43 1: 54–64.
  73. 73. Orejas M, Espeso EA, Tilburn J, Sarkar S, Arst HN Jr, et al. (1995) Activation of the Aspergillus PacC transcription factor in response to alkaline ambient pH requires proteolysis of the carboxy-terminal moiety. Genes Dev 9 13: 1622–32.
  74. 74. Bradford MM (1976) A rapid and sensitive method for the quantitation of microgram quantities of protein utilizing the principle of protein-dye binding. Anal Biochem 72 248–54.
  75. 75. Schrettl M, Bignell E, Kragl C, Joechl C, Rogers T, et al. (2004) Siderophore biosynthesis but not reductive iron assimilation is essential for Aspergillus fumigatus virulence. J Exp Med 200 9: 1213–9.
  76. 76. Saijo S, Fujikado N, Furuta T, Chung SH, Kotaki H, et al. (2007) Dectin-1 is required for host defense against Pneumocystis carinii but not against Candida albicans. Nat Immunol 8 1: 39–46.
  77. 77. Huang DW, Sherman BT, Lempicki RA (2008) Systematic and integrative analysis of large gene lists using DAVID bioinformatics resources. Nat. Protocols 4 1: 44–57.
  78. 78. Huang DW, Sherman BT, Lempicki RA (2009) Bioinformatics enrichment tools: paths toward the comprehensive functional analysis of large gene lists. Nucleic acids research 37 1: 1–13.
  79. 79. Walker LA, Munro CA, de Bruijn I, Lenardon MD, McKinnon A, et al. (2008) Stimulation of chitin synthesis rescues Candida albicans from echinocandins. PLoS Pathog 4 4: e1000040.
  80. 80. Mora-Montes HM, Netea MG, Ferwerda G, Lenardon MD, Brown GD, et al. (2011) Recognition and blocking of innate immunity cells by Candida albicans chitin. Infect Immun 79 5: 1961–70.
  81. 81. Plaine A, Walker L, Da Costa G, Mora-Montes HM, McKinnon A, et al. (2008) Functional analysis of Candida albicans GPI-anchored proteins: roles in cell wall integrity and caspofungin sensitivity. Fungal Genet Biol 45 10: 1404–14.
  82. 82. Wheeler RT, Fink GR (2006) A drug-sensitive genetic network masks fungi from the immune system. PLoS Pathog 2 4: e35.
  83. 83. Fujikawa T, Kuga Y, Yano S, Yoshimi A, Tachiki T, et al. (2009) Dynamics of cell wall components of Magnaporthe grisea during infectious structure development. Mol Microbiol 73 4: 553–70.
  84. 84. Gravelat FN, Ejzykowicz DE, Chiang LY, Chabot JC, Urb M, et al. (2010) Aspergillus fumigatus MedA governs adherence, host cell interactions and virulence. Cell Microbiol 12 4: 473–88.
  85. 85. Towbin H, Staehelin T, Gordon J (1979) Electrophoretic transfer of proteins from polyacrylamide gels to nitrocellulose sheets: procedure and some applications. Proc Natl Acad Sci U S A 76 9: 4350–4.