Homeostatic maintenance and age-related functional decline in the Drosophila ear

Abstract

Age-related hearing loss (ARHL) is a threat to future human wellbeing. Multiple factors contributing to the terminal auditory decline have been identified; but a unified understanding of ARHL - or the homeostatic maintenance of hearing before its breakdown - is missing. We here present an in-depth analysis of homeostasis and ageing in the antennal ears of the fruit fly Drosophila melanogaster. We show that Drosophila, just like humans, display ARHL. By focusing on the phase of dynamic stability prior to the eventual hearing loss we discovered a set of evolutionarily conserved homeostasis genes. The transcription factors Onecut (closest human orthologues: ONECUT2, ONECUT3), Optix (SIX3, SIX6), Worniu (SNAI2) and Amos (ATOH1, ATOH7, ATOH8, NEUROD1) emerged as key regulators, acting upstream of core components of the fly’s molecular machinery for auditory transduction and amplification. Adult-specific manipulation of homeostatic regulators in the fly’s auditory neurons accelerated - or protected against - ARHL.

Introduction

A surface calm can be misleading. All living things, from unicellular amoeba to neurons in the human brain, require continual maintenance and the constant flow of their seemingly equable physiological operations is in fact the product of complex homeostatic networks. All life, it has been said, needs to run to stand still. As with many things, the underlying machinery remains largely unrecognized until it breaks down. A most pertinent example of such a breakdown are the hearing impairments that affect about 1.23 billion people worldwide, corresponding to one sixth of the world’s total population1. The aetiology of hearing loss is diverse but the arguably single most important factor is age. Age-related hearing loss (ARHL) carries the vast bulk of the global disease burden, but no treatments, neither preventive nor curative, are currently in sight. Multiple factors have been linked to ARHL, including extrinsic (e.g. noise exposure, ototoxic drugs or smoking) as well as intrinsic (molecular, physiological) ones2,3,4. Over the past few decades, gene discovery studies using mouse models have also identified numerous candidate genes for human deafness5,6,7,8,9,10,11. Three recent larger scale screens in mice and one recent genome-wide association screen (GWAS) in humans have brought the total number of candidate hearing loss genes to 15412,13,14,15. Yet, a unified view on the underlying mechanisms of ARHL, and particularly the gene-regulatory networks that mediate the maintenance of sensitive hearing throughout the lifespan, is still lacking. We here use the auditory system of the fruit fly in an attempt to shed some light on these issues.

Despite the stark anatomical differences, the ears of vertebrates and Drosophila also share marked similarities; these include (i) some fundamental biophysical mechanisms of auditory transduction16 and amplification17,18, (ii) the fact that the inner ears of flies and vertebrates host the sensors for both sound and gravity and that these also display a broadly similar architecture of neuronal pathways from the ear to higher-order centres in the brain19 and, finally, (iii) molecularly conserved families of proneural genes that control hearing organ development, such as e.g. ato20 in flies and Math1/Atoh1 in mice (or ATOH1 in humans)21. The various similarities and – molecularly - near identities22,23, between the ears of Drosophila and vertebrates (including mammals) have recommended the fly as a powerful model to study more fundamental aspects of hearing and deafness24, especially those around transducer-based amplification, which are facilitated in Drosophila due to their lack of both Prestin-mediated electromotility25 and efferent innervation26.

Many Drosophila hearing genes have been identified24,27,28, but so far no study has explored the flies’ hearing across their life course. We found that the ears of fruit flies also display ARHL; virtually all parameters of sensitive hearing start declining after 50 days of age (at 25 °C).

Taking one step back, however, we set out to identify those homeostatic regulators that maintain the fly’s sensitive hearing before the onset of ARHL. We combined RNA-Seq-based transcriptomics with bioinformatical, biophysical and behavioural tools to explore the landscape of age-variable genes of the Johnston’s Organ (JO) - the flies’ inner ear’. Our data suggests that the thereby identified transcriptional regulators are not restricted to Drosophila - or the sense of hearing - but represent key players of homeostasis across taxa and possibly across sensory modalities.

Results

Drosophila is prone to age-related hearing loss (ARHL)

Functionally, the Drosophila antennal ear (Fig. 1a) comprises of two components: (i) the external sound receiver (jointly formed by the third antennal segment, A3, and its lateral appendage, the arista) and (ii) the actual ‘inner ear’, which is formed by Johnston’s Organ (JO), a chordotonal organ29 located in the second antennal segment, A2. JO harbours ~500 mechanosensory neurons30.

Figure 1
figure1

Drosophila Hearing across the life course. (a) Schematic representation of Johnston’s Organ (JO), a chordotonal organ located in the 2nd antennal segment. JO harbours the mechanosensory units (scolopidia) that mediate the sensation of sound in Drosophila. Sound waves act on the feathery arista, forcing the 3rd antennal segment to rotate about its longitudinal axis, thereby stretch-activating specialised mechanosensory ion channels (Nan, Iav, NompC) in the scolopidial neurons. (b) Sound-evoked activity (shown in light blue, male locomotor responses to courtship song, seen in 10-day and 50-day old flies (p < 0.001 in both, paired t-test) are abolished in 60-day old flies. Baseline activity levels (shown in grey, male locomotor activity when not stimulated) are not significantly different between 10 and 60 day old flies. [p = 0.487, t-test; sample sizes: n(day 10) = 12, n(day 50) = 10, n(day 60) = 14]. (c) Power Spectral Densities of unstimulated antennal sound receivers betray age-related decline of hearing in both males (left, shades of blue) and females (right, shades of red). Preceded by homeostatic oscillations around their baseline values, all principal parameters of hearing (shown in right-hand panels for both sexes) indicate a loss of hearing from day ~50 onwards: the receiver’s best frequency starts rising towards the level of the passive system, the auditory energy gain drops to near zero and tuning sharpness falls to values around ~1. [sample sizes males: n(day 1) = 18, n(day 5) = 13, n(day 10) = 6; n(day 25) = 19, n(day 50) = 16), n(day 60) = 11, n(day 70) = 18; sample sizes females: n(day 1) = 17, n(day 5) = 8, n(day 10) = 4; n(day 25) = 17, n(day 50) = 20), n(day 60) = 12, n(day 70) = 17]. (d) Mechanical and electrophysiological responses to force steps allowed for probing JO mechanotransducer function across the auditory life course in male (left, blue) and female (right, red) flies. Mechanical integrity of auditory transducers was quantified by fitting gating spring models to the antennal receiver’s dynamic stiffness (slope stiffness) as a function of its peak displacement (see ref.16 for details). Electrophysiological function was assessed by recording compound action potential (CAP) responses from the antennal nerve. CAP responses showed an identical pattern across the life course in both males and females: CAP response magnitudes substantially increased from day 1 to day 25, then monotonously declined from day 25 to day 70. The largest drop in CAP magnitudes occurred between day 50 and day 70, with responses of 70-day-old flies even falling below those of 1-day-old flies. Transducer mechanics, in contrast, remained more intact throughout. However, at day 70 the four principal parameters of transducer function, i.e. the number of sensitive transducer channels Ns), the number of insensitive transducer channels (Ni), the sensitive single channel gating force (zs) and the insensitive single channel gating force (zi) were all significantly different from their values at day 1, in both males and females (Mann-Whitney U test, p < 0.01 for all). Interestingly, no such change was observed for the stiffness of the antennal joint (Ksteady), which is a transducer-independent measure of antennal mechanics. Next to these properties shared between males and females, our analyses also revealed some sexually dimorphic phenomena: KGS was significantly different only in males (Mann-Whitney U test, p < 0.01). Whereas in females Ns, Ni, zs and zi, remain at constant values until the age of 50 days, the respective values of male flies change monotonously throughout the life course, with continually falling numbers of transducer channels being compensated by increasing single channel gating forces (thereby homeostatically balancing the male antenna’s nonlinear stiffness). [all error bars are SEM; sample sizes males: n(day 1) = 8, n(day 25) = 10, n(day 50) = 10), n(day 70) = 8; sample sizes females: n(day 1) = 11, n(day 25) = 10, n(day 50) = 10), n(day 70) = 7].

To assess hearing across the Drosophila life course we first measured the locomotor activities of flies in response to a playback of courtship song components at different ages. Drosophila melanogaster males increase locomotor activity in response to courtship song31. While 10- and 50-day-old flies increased their locomotor activity in response to a 15 min long train of courtship song pulses (inter-pulse-interval, IPI: 40 ms), sound-induced responses were absent in 60-day-old flies (Fig. 1b, left). We did, however, observe courtship behaviour (wing extension) in 60-day old males when paired with younger virgin females (data not quantified); consistent with this, so far no study has reported a cut-off age for male mating drive in Drosophilid flies. While individual parameters of male mating performance decline with age32; other parameters appear to increase33, suggesting that the observed loss of response is not a loss of mating interest per se. Moreover, baseline locomotor activities of 60-day-old flies were the same as in 10-day-old flies (Fig. 1b, right), pointing towards an auditory - rather than a more generalised neurological - deficit as the underlying cause for the non-responsiveness to sound.

A simple, but quantitatively powerful, test of auditory performance was then conducted by recording the vibrations of unstimulated sound receivers (free fluctuations)18. A receiver’s free fluctuations reveal three principal parameters of auditory function: (1) the ear’s best frequency, f0 (measured in Hz), (2) its frequency selectivity or quality factor, Q (dimensionless), and (iii) its energy - or power - gain (measured in KBT). Much like hair cells in the vertebrate inner ear, the antennal ears of Drosophila are active sensors, which inject energy into sound-induced receiver motion34.

Our data show that the ears of flies, much like those of humans, show age-related hearing loss (ARHL) (Fig. 1c). At 25 °C, the antennal receivers of 70-day-old flies show (i) best frequency shifts towards the passive system, where no energy injection is observed, (ii) a greatly reduced tuning sharpness and (iii) a ~90% loss of their energy gains (Fig. 1c and Supplementary Table 1), indicating a near-complete breakdown of the active process - which supports hearing - at day 70. The time course of this auditory decline was broadly similar between males and females (Supplementary Table 1).

To probe auditory function in more detail, we also quantified the mechanical and electrophysiological signatures of auditory mechanotransduction in response to force-step actuation of the fly’s antennal ear at different ages (Fig. 1d). Direct mechanotransducer gating introduces characteristic nonlinearities - namely drops in stiffness - into the mechanics of the sound receiver. These so-called ‘gating compliances’ can be modelled with a simple gating spring model16,35 thereby allowing for calculating the number - and molecular properties - of different populations of mechanosensory ion channels present in the fly’s JO36. Two distinct mechanotransducer populations have previously been described: a sensitive population, linked to hearing, and an insensitive population, linked to the sensation of wind and gravity19. At day 70, the numbers of predicted sensitive (Ns) and insensitive (Ni) channels have decreased by ~50% as compared to their values at day 1; the single channel gating forces of the sensitive (zs) and insensitive channels (zi), in turn, have increased (Fig. 1d). The receiver’s steady-state stiffness (Ksteady), however, which is an indicator of the integrity of the antennal joint, is not significantly different between 1- and 70-day-old flies, suggesting that the changes in auditory mechanics reflect an ageing of the mechanotransducer machinery rather than structural changes of the organ itself. Compound action potential (CAP) responses to force step actuation - recorded from the antennal nerve - showed that nerve response magnitudes initially increased from day 1 to day 25 and then decreased steadily, with response curves of 70-day-old flies falling below those of 1-day-old flies, both in response magnitude and displacement sensitivity (Fig. 1d). The above-described pattern of transducer ageing was seen in both males and females. Some subtle differences, however, could be observed between the sexes. While females displayed a ~stable baseline of most transduction parameters up to day 50, males showed signs of a steadier decline from day 1 on. Also, gating spring stiffnesses (KGS) decreased in 70-day-old males but increased in 70-day-old females (Fig. 1d).

Summing up the behavioural, mechanical and electrophysiological evidence, the auditory life course of Drosophila melanogaster can roughly be broken down into two phases: (i) a dynamic phase of homeostatic metastability, which is characterised by fluctuations of key parameters of hearing around a ~stable baseline, and which lasts from day 1 to ~day 50 (also including possible signs of initial functional maturation) and (ii) a phase of terminal decline, which starts at ~day 50 and leads to a near complete loss of auditory function at ~day 70.

We hypothesized that a breakdown of the homeostatic machinery, which shapes auditory performance during the life course and maintains healthy hearing up until day 50, might be the ultimate reason for the observed terminal decline. In order to identify the molecular networks involved, we therefore profiled the auditory transcriptome at days 1, 5, 10, 25 and 50 through RNA sequencing (RNA-Seq) of the 2nd antennal segment (Supplementary Table 2).

The age-variable auditory transcriptome in Drosophila

16,243 genes are expressed in the 2nd antennal segment in both males and females (Supplementary Table 2); 13,324 of those are protein-coding. We compared the expression levels of all genes in a pair-wise manner, between (i) day 1 and 5, (ii) day 5 and 25 and (iii) day 25 to 50. In total, 5,855 (4,936 protein-coding) genes were changing their expression significantly in at least in one of the three pair-wise comparisons (criteria: >1.5-fold change; <10% False Discovery Rate (FDR); p < 0.05; Supplementary Table 3 and Supplemental Methods). This first step of the analysis identified those genes that showed a significant change of expression level at any stage of the life course, irrespective of the corresponding sign of this change (up- or downregulation). 64% of all genes (10,388 of 16,243) showed constant expression levels and were ruled out at this stage.

The gene-ontological nature of age-variable genes in A2 was probed with the Gene Ontology enRIchment anaLysis and visualization (GOrilla) tool37,38. The age-variable transcriptome revealed both down- and upregulation of genes. Genes involved in ATP metabolism, protein processing and structural molecules were found to be downregulated, whereas immune response genes, photo transduction genes and translation machinery genes were upregulated (Fig. 2a and Supplementary Table 4). Next to many novel JO genes, about one third (109) of all previously reported JO genes (314)24,28 changed their expression in our dataset (Table 1); this included rhodopsins, the TRPV channel gene nan, innexins, as well as ATPase β subunits (nervanas) previously linked to JO function39,40.

Figure 2
figure2

Gene-Ontology and Bioinformatics of the Drosophila age-variable JO transcriptome. (a) Gene Ontology (GO) based summary of age-variable genes in JO as derived from RNAseq data taken across different age points (days 1, 5, 10, 25 and 50). Down-regulated (blue) and up-regulated (red) genes from multiple pairwise comparisons between all age points are shown on the left and right side of the graph, respectively. The bubble diameter is proportional to the gene number (the larger the diameter the more genes were down -or up-regulated. The y-axis shows numbers of the genes and the x-axis the Log2Fold-Change (Log2FC) of gene expression. GO terms correspond to the up-regulated (right) or down-regulated (left) genes, a selection of which is shown in the respective neighbouring boxes; enrichment scores are shown in brackets. Selection of the most age variable genes are shown in individual boxes corresponding to each GO term next to it. Individual bubbles denote the number of genes (y-position of bubble centre) and their corresponding range of Log2FC values; negative ranges like ‘−1 < x < −0.59’ mean that genes were downregulated between 21 and 20.59 times, whereas positive ranges like ‘1 < x < 0.59’ denote an upregulation between 21 and 20.59 times. (b) Prediction of upstream transcriptional master regulators for age-variable JO target genes (based on motif-binding analysis in the iRegulon software package). Identified master regulators wor, amos, Optix and onecut are shown in yellow with arrows leading to their predicted targets. Targets are grouped, up and down-regulated genes shown in blue and red, respectively. Mechanosensory ion channels, previously linked to fly hearing, are shown in green: iav and nompC are predicted to be downstream of onecut, amos and Optix, whereas nan is predicted to be downstream of wor, Optix and onecut.

Table 1 Previously identified JO genes with age-variable expression.

We also found that 67% (74 out of 111) of hearing loss genes recently identified in mice12,13,14 are conserved in flies - and expressed in A2 – with 32% of them also showing age-variable expression in JO. In addition, a recent genome-wide association screen (GWAS) identified 44 new genes associated with ARHL in humans; 80% of those are conserved in flies - and expressed in A2 – with 27% being age-variable15 (Table 2).

Table 2 Mouse genes linked to deafness, which are conserved - and expressed - in the Drosophila JO.

Number of JO neurons remains constant up until the age of 50 days

To test whether the age-variable transcriptome between day 1 and day 50 reflected changes on the cellular level we counted the number of neurons in the second antennal segment at different ages (Supplementary Fig. 1). From day 1 to day 50 no difference in neuronal numbers was seen, suggesting that the observed transcriptomic changes betray an age-variable transcriptional - i.e. gene-regulatory - activity.

Predicting the gene-regulatory landscape of auditory homeostasis in Drosophila

In order to shed light on the gene-regulatory networks of auditory homeostasis and identify key transcription factors (TFs) acting upstream of the age-variable genes, we applied the bioinformatics software package iRegulon, which predicts TFs based on motif binding probabilities41.

Our heuristic rationale was based on three assumptions: (i) auditory homeostasis involves, at least in parts, specific TFs; (ii) TFs can be low abundance genes, their action can be mediated through small changes in expression levels; (iii) every TF has, on average, more than one target and those targets might be functionally, or gene-ontologically, linked.

We drew three consequences from the above premises: First, we concentrated our study on TFs. Second, we used the entire age-variable auditory regulon to predict upstream TFs, thereby increasing the overall sensitivity of our analysis. Even TFs, which might have escaped our attention from the RNA-Seq data itself could thus be recovered in subsequent bioinformatical analyses. Third, we grouped putative regulons (i.e. subsets of expressed genes) not only by their variability with age but also by their gene-ontological classification.

37 TFs were predicted from different rounds of gene submission (Supplementary Table 5), based on varying gene ontological categories, such as (i) transporters and receptors, (ii) trafficking genes, (ii) structural genes, (iv) most abundantly expressed genes or (v) genes most variable between ages (Fig. 2b). Onecut, Optix, atonal (ato), Drop (Dr), cubitus interruptus (ci), Sox100B and PvuII-PstI homology 13 (Pph13) were predicted to regulate the transcription of receptors and transporters, including the key auditory ion channels NompC and Nanchung (Nan). Absent MD neurons and olfactory sensilla (amos) and Optix were predicted to regulate the transcription of structural genes, such as actins and tubulins (the most severely downregulated genes (Fig. 2a). Worniu (wor) was predicted to be upstream of trafficking machinery, while amos and wor were both upstream of dynein motor proteins, which are indispensable for ion channel transport and homeostasis (Supplementary Fig. 2).

Testing predicted homeostatic regulators of Drosophila hearing

To test the validity, and functional relevance, of the bioinformatical analyses, we used RNAi-mediated, adult-specific knockdowns (KDs) of 19 (out of 37) predicted transcription factors: Adult enhancer factor 1 (Aef1), absent MD neurons and olfactory sensilla (amos), anterior open (aop), araucan (ara), atonal (ato), cut (ct), glass (gl), longitudinals lacking (lola), onecut, Optix, pannier (pnr), PvuII-PstI homology 13 (Pph13), regulatory factor X (Rfx), runt (run), Sox box protein 14 (sox14), serpent (srp), Signal-transducer and activator of transcription protein at 92E (Stat92E), TATA-binding protein (Tbp) and worniu (wor) (Supplementary Table 6). The adult-specific knockdown was achieved by using a neuron-specific Gal4 driver line in combination with a temperature-sensitive transcriptional inhibitor of Gal4 (Gal80ts) and the respective UAS-RNAi constructs. Transcription of RNAi constructs was initiated by transferring flies to a 30 °C environment post eclosion. RNAi efficacy was validated by means of RT-qPCR and showed at least 60% reduction of gene expression (Supplementary Fig. 3). Analysing the free fluctuations of the antennal sound receiver, we found 5 cases (onecut, amos, gl, lola and Sox14), where the knockdown accelerated the ARHL phenotype; 4 other cases (wor, Optix, Pph13 and ara), however, showed protective phenotypes for various principal parameters of auditory function (Supplementary Table 6). Adult-specific knockdowns of the crucial developmental genes ato20, Rfx42 and ct43 did not show any significant phenotypic changes (Supplementary Table 6), suggesting that they are not involved in homeostatic maintenance of hearing in adults.

To get a better understanding of the specific TF-mediated homeostatic programme that maintains hearing, we concentrated on the top four regulators, which occurred consistently throughout various rounds of bioinformatical analyses. These were onecut, Optix, wor and amos, all of which showed clear expression in the neurons of JO (Fig. 3). These four TFs also showed the strongest KD phenotypes in the free fluctuation experiments (Fig. 4a,b and Supplementary Table 6), with each TF affecting distinct aspects of auditory function. Analysing the mechanical and electrophysiological signatures of mechanotransducer gating across the four KDs (Fig. 4c,d) identified onecut as a crucial homeostatic regulator of auditory transducer function. The number of predicted sensitive (auditory) transducer channels (Ns) is greatly reduced in onecut KD flies, while their single channel gating forces (zs) are increased. The numbers of predicted insensitive (non-auditory) channels (Ni) are slightly increased and their single channel gating forces (zi) decreased in onecut KDs. The observed inverse relationship between ion channel numbers and gating forces might represent an intrinsic homeostatic link between the two parameters (see also discussion and Supplementary Fig. 4). CAP responses to force-step actuation, finally, are dramatically reduced in the KD condition. The overall effect of the adult-specific KD of onecut is a near-complete abolition of the mechanical and electrical signatures of sensitive auditory transducer gating. Consistent with these results, onecut KD flies specifically lose their responsiveness to sound, while their baseline locomotor activities remain unchanged (Fig. 4e). KDs of Optix, amos and wor showed less pronounced effects on electrophysiological or mechanical signatures of transducer gating, but at least one transducer parameter was affected in each genotype (Fig. 4d). Similarly to onecut KD, amos KD flies lose their responsiveness to sound, whereas KD of wor and Optix increases the sensitivity to sound, which manifests in an acoustic startle, i.e. a reduction of activity in response to sound (Fig. 4e). For three of the four master regulators (Optix, wor, amos), overexpression constructs were available, we thus also explored whether overexpression could invert the knockdown phenotypes seen in the free fluctuation analyses (compare to Fig. 4a); this was indeed the case for Optix and amos (Supplementary Fig. 5); wor overexpression was indistinguishable from controls (Supplementary Table 6). Canton-S flies show accelerated age-related hearing loss (aARHL) at 30 °C, their hearing loss after 25 days is equivalent to that of 60-day-old flies raised at 25 °C. Over-expression of amos or downregulation of wor (both 30 days at 30 °C) - led to a partial prevention of the age-related auditory decay (Fig. 5c).

Figure 3
figure3

Expression validation of homeostatic master regulators in JO. All four predicted regulators (Wor, Amos, Optix and Onecut) are expressed in JO (expression analysis was done at the age of day 10 for all genotypes). Expression of Wor was detected by expressing EGFP under the control of a wor-Gal4 driver; expression of Amos, Optix and Onecut was detected by using GFP-tagged flyFos gene expression constructs78. Co-labelling with antibodies against two pan-neuronal markers (the nuclear marker Elav, red; and the membrane marker HRP, blue) confirmed neuronal expression for all four regulators. Arrowheads indicate examples of clear co-localization between the three signals.

Figure 4
figure4

Functional validation of homeostatic master regulators. (a) Average vibration velocities of female unstimulated sound receivers (‘free fluctuations’) after adult-specific, RNAi-mediated knockdown (KD; red solid lines) for all four master regulators alongside their respective controls (grey dashed lines). KDs of amos and onecut show a loss of sound receiver function, as evident from (i) reduced energy content (‘power gain’), (ii) reduced frequency selectivities, and - in the case of onecut - also (iv) best frequency shifts towards higher values. KDs of wor and Optix, in contrast, show enhanced sound receiver function, as evident from (i) increased energy content and (ii) increased frequency selectivity (wor) or best frequency shifts to lower values (Optix). [Supplementary Table 6 for numerical details and statistics]. All flies were assessed 15 days after eclosion. (b) Line plot summaries comparing the KD sound receiver phenotypes [as from (a)] to the sound receiver phenotypes occurring naturally during ageing (reference for comparison: Canton-S day 1 to day 70). Arrows indicate significant changes in parameters. Black arrows indicate that KD phenotypes (relative to their corresponding controls) phenocopy the age-related hearing loss (ARHL) phenotypes seen in wildtype flies. White arrows indicate a reversal of the specific ARHL phenotype. (c) Gating compliances (average fits, top) and CAP responses (medians plus standard errors, bottom) to force step actuation across adult-specific KDs of four master regulators (red) and their corresponding controls (grey). CAP responses are plotted against both stimulus force and antennal displacements. KD of onecut leads to a dramatic loss of auditory transducer function, as evident from the near complete loss of the gating compliance for the most sensitive transducers and the loss of nerve responses to small stimulus forces/displacements. KDs of wor, amos and Optix have subtler effects on transducer mechanics but all reduce nerve responses to larger stimulus forces/displacements. (d) Line plot summaries of transducer mechanics [from (C)] in four regulator KDs (red) relative to controls (green). Dashed lines indicate respective control values. Significant changes are asterisked (*). (e) Sound-induced behavioural responses in males after wor, amos, Optix and onecut KD (red) compared to control flies (grey). wor KD mutants show hypersensitivity to sound and show significant reduction of locomotor activity to sound compared to the baseline (n = 14,p = 0.029, Mann-Whitney Rank Sum Test), amos KD mutants do not respond to sound (n = 12, p = 0.503, t-test), Optix KD mutants show hypersensitivity to sound and show significant reduction of locomotor activity to sound compared to the baseline (n = 17,p = 0.001, Mann-Whitney Rank Sum Test), onecut KD mutants do not respond to sound (n = 10, p = 0.277, t-test), while their respective controls show an increase in locomotor activities in response to sound (n = 36, p = <0.001, Mann-Whitney Rank Sum Test).

Figure 5
figure5

Key molecular targets validation and gene therapeutic approach to ARHL. (a) Gene expression changes after regulator KDs as quantified by RT-qPCR. wor and amos KDs show significant reduction of the dynein motor Dhc98D, while KD of Optix leads to overexpression of NompC; onecut KD reduces expression of both nan and iav. (n indicates the biological replicates, error bars show standard deviations, *p > 0.05, **p > 0.01). (b) Vibration velocity of the sound-receiver and the sharpness of the tuning Q are significantly reduced in Dhc98D knockdown flies (shown in red) compared to the controls (shown in dotted grey). See also Supplementary Table 6. (c) Power Spectral Densities of unstimulated antennal sound receivers betray accelerated age-related hearing loss (aARHL) in flies kept at 30 °C (left), with a near complete loss of receiver activity already at ~day 25 (light blue area: 1 day old flies; dark blue area: 25 day old flies). A 30-day-long amos (middle) overexpression (OE) or wor (right) knockdown (at 30 °C) protects receivers from the age-related loss of activity (dark blue: KD or OE, respectively; light blue: controls). Box plots show energy contents (power gains) for each transgenic intervention (dark blue) relative to controls (light blue).

qPCR validation reveals key auditory targets of master regulators

Knockdown and overexpression of identified homeostatic TFs altered important parameters of the fly’s ear, such as its frequency tuning, mechanotransduction, amplification and nerve responses (Fig. 4a–d). All of these system properties are thought to arise from an interaction of three key transient receptor potential (TRP) channels, namely Nanchung (Nan)44, Inactive (Iav)45 and NompC46 with motor proteins from the dynein family27. One such dynein was also identified within our age-variable gene set, this is the Dynein heavy chain at 98D (Dhc98D). The three TRP channels from above, as well as the auditory dyneins were predicted downstream of the four master regulators (Fig. 2b, Supplementary Fig. 2). Using real-time quantitative polymerase chain reactions (qPCRs) we therefore tested if nan, iav, nompC and Dhc98D levels were under the control of the identified homeostatic TFs (Fig. 5a). RNAi-mediated adult-specific knockdown of onecut resulted in a dramatic downregulation of both nan and iav, knockdown of Optix lead to an upregulation of nompC levels, whereas knockdown of amos and wor showed downregulation of Dhc98D.

Adult-specific knockdown of Dhc98D caused a strong hearing loss phenotype similar to the one seen after amos KD (Figs. 4a and 5b).

Discussion

We show that flies, just like humans, are prone to age-related hearing loss (ARHL). ARHL manifests in various aspects of Drosophila hearing function. As remarkable as its eventual decay, however, is the long period (~50 days) during which sensitive hearing is preserved. We probed the molecular bases of this homeostatic preservation. The specific environmental conditions of our ageing cohorts (see methods for details) meant that antennal stimulations occurring during the flies’ life course were almost exclusively caused by the animals’ own locomotion, thereby approximating the minimal noise floor possible for freely moving, intact flies. Our study thus explored the gene regulatory network of auditory homeostasis in acoustically unchallenged ears.

Across taxa, ears are delicate mechano-electrical converters. Their operation can be conceptually divided in a passive and an active component. Both with regard to its natural life course and the effects of our transgenic manipulations the steady-state stiffness, Ksteady (a good indicator of the passive oscillator16) - remained one of the most stable parameters of auditory function (Figs. 1d and 4d), suggesting that the causes for the functional decline emerge from the active system. The active oscillator of the fly’s ear emanates from its auditory transducer modules, i.e. mechanosensory ion channels that act in series with – and receive feedback from17 – probably dynein-based motor proteins27. This functional design explains vast parts of the functional performance of the Drosophila ear17; its quantitative modelling also allows for extracting vital parameters of auditory function, such as the amount of energy that auditory neurons inject into the hearing process or the number – and molecular properties – of transducer channels they harbour.

Quantitatively, the hearing loss observed in flies older than 50 days is best described as a loss of power gain (Fig. 1c), i.e. a loss of the active, transducer-based process by which auditory neurons amplify sound-induced motions of the antennal sound receiver. Comparing the rather sharp drop of the flies’ auditory life span to their survival rates reveals a close alignment of the two time courses (Fig. 6). This suggests that the - metabolically costly - operations of the homeostatic network have evolved to maintain function up to the expected lifespan but not beyond. Such behaviour has been predicted by the ‘disposable soma’ theory of ageing47,48, which postulates that an organism’s investment in somatic maintenance will not exceed its reproductive period48; the dissociation between healthspan and lifespan observed in today’s human societies, and evidenced not least by ARHL, lies at the heart of these evolutionary relations.

Figure 6
figure6

Comparison of lifespan and auditory healthspan. The flies’ auditory health span (here depicted as median auditory gain in % of its maximum value) and survival rates (three independent cohorts shown) are closely aligned. Both show sharp drops from ~50 days on (stocks kept at 25 °C and 60% relative humidity).

The flies’ age-related loss of auditory power gain is accompanied by a gradual loss of nerve response (CAP amplitudes), which decline steadily from day 25 already, in both males and females, potentially indicating a progressive neuropathy (Fig. 1d). This shows that ageing occurs on various levels of auditory function, including transduction, motor-based feedback amplification and signal transformation into action potential responses. Auditory transducers, however, also display a remarkable resilience throughout life; the characteristic nonlinear signatures they introduce into sound receiver mechanics (gating compliances) stay broadly constant up to the age of 70 days (Fig. 1d). First quantitative gating spring model analyses also hint at a possible homeostatic mechanism for this constancy: In both males and females, and across ages, transducer channel numbers were found to be inversely correlated with their respective single channel gating forces. When transducer numbers decrease with age, their single channel gating forces increase, thereby stabilizing the nonlinear mechanics of the sound receiver across the auditory life course (Supplementary Fig. 4). This homeostatic stabilization of receiver nonlinearity is particularly significant, as all changes in receiver mechanics will affect all neurons and thereby global JO function. In order to understand these, and other, homeostatic mechanisms we explored the transcriptional network that mediates them.

We found that 16,243 genes are expressed in the 2nd antennal segment, which harbours the fly’s inner ear (JO); 5,855 out of these change their expression in at least one of the pair-wise age comparisons. Four transcription factors emerged from our bioinformatical analysis as key regulators of the age-variable auditory transcriptome, all of which are conserved in the human genome; these are Onecut, Worniu, Optix and Amos.

Onecut is a transcription factor known to be involved in photoreceptor differentiation in flies49 and retinal ganglion cell development in mice, where it cooperates with Pou4f2 (acj6) and Atoh7 (closest fly orthologues: ato, amos)50. We here report an essential role for Onecut in fly hearing or - more precisely – in the homeostatic maintenance of fly hearing. An adult-specific knockdown (KD) of the onecut gene across JO neurons affects all levels of auditory system function and leads to deafness. The onecut KD phenotype includes near complete losses of auditory (i) transducer gating, (ii) amplification and (iii) nerve responses, as well as (iv) a loss of sound-evoked behaviour. A first probing of possible Onecut targets through qPCR in onecut KD flies (Fig. 4f) might reveal one possible mechanism of action, which is the direct transcriptional regulation of the two interdependent TRPV channels Nan and Iav. Nan/Iav are thought to form a heterodimeric ion channel specifically in chordotonal neurons. Both genetic44,45 and pharmacological51 ablations of Nan/Iav channels have been shown to eliminate chordotonal mechanosensory function. After an adult-specific knockdown of onecut, JO expression levels of both nan and iav showed a dramatic decline. This downregulation coincided with a near complete abolition of the gating compliances associated with sound-sensitive neurons, indicating a failure of auditory transduction. A total loss of transducer function would also be sufficient to explain the effects on auditory amplification and nerve responses observed further downstream the auditory signalling chain. Intriguingly, onecut was also predicted to be upstream of the kinesin-dependent machinery for anterograde transport in chordotonal cilia (Supplementary Fig. 7a). The observed total absence of Iav expression in JO after onecut KD (Supplementary Fig. 7b) could thus be the combined result of a reduced transcription (see Fig. 5a) and a defective ciliary transport, which requires kinesin activity. Interestingly, both Nan/Iav44,45,52, as well as NompC53,54, have previously been proposed as auditory transducer components in Drosophila. Further studies also demonstrated beyond doubt that NompC contains all elements required to form a bona-fide mechanotransducer channel55,56. In contrast to nan/iav, however, nompC transcript levels in JO remained unchanged after onecut KD.

worniu (wor) is a zinc finger transcription factor that belongs to the Snail family. We here demonstrate that adult-specific down-regulation of wor enhances auditory amplification and sharpens auditory tuning. These effects are sustained up until 30 days of downregulation (at 30 °C) - when the ears of control flies already show a near complete loss of power gain - suggesting that knockdown of worniu can protect distinct aspects of auditory function from their age-dependent decline. Genes previously reported to be upregulated in wor mutants included cadherins and trafficking proteins, e.g. Rabs57; our bioinformatics prediction also support a role of wor in the regulation of the cellular trafficking machinery (Supplementary Fig. 2). In JO, the adult-specific KD of wor had virtually no effect on auditory transducer gating or the transformation of antennal motion into nerve responses. Auditory amplification and tuning sharpness, however, were significantly enhanced in wor KD flies; both of these parameters are linked to the dynein-based motor machinery that acts in series with the auditory transducer channels. Consistent with these mechanistic considerations, qPCR analyses of the JOs of wor KD flies showed a downregulation of Dhc98D; neither nompC, nan nor iav levels were affected.

Optix belongs to the sine oculis homeobox (SIX) family of transcription factors and is required for eye formation58. The adult-specific knockdown of Optix in JO neurons leads to an increase in the receiver’s power gain and a shift of its best frequencies to lower values, both indicative of more active system. qPCR analyses showed that these changes in auditory activity coincided with an upregulation of nompC. These relations are consistent with the reported roles of NompC in auditory amplification46. Auditory transducer gating, however, was not affected; both numbers and single channel gating forces of sensitive auditory transducers were identical between the ears of Optix KDs and control flies. Also, CAP responses to small antennal displacements (as caused by auditory stimuli) were unchanged. CAP responses to larger displacements (as caused by non-auditory stimuli), in contrast, were decreased as compared to controls. This suggests a more complex role of Optix in the homeostatic regulation of auditory, as well as non-auditory populations of JO neurons.

amos is a proneural gene from the family of basic-helix-loop-helix (bHLH) transcription factors. bHLH transcription factors also include ato, which specifies chordotonal organs20,59, R8 photoreceptor precursors59,60, and a subset of olfactory sense organs61. amos specifies two other subsets of olfactory sense organs and a mechanosensory subset of larval bipolar dendritic neurons62,63. Ato and amos share a high sequence similarity in their bHLH domains (73% amino acid identity) and their basic - DNA-binding - regions are identical. Maung and Jarman showed that amos is capable to rescue eye development independent of ato64. Weinberger et al. showed that the coding sequence of amos, when used to replace the coding sequence of ato, is sufficient to produce a fully functional Drosophila ear, the performance of which is statistically identical to the native, ato-induced organ with respect to all quantitative parameters also used in this study23. While amos was found to be expressed in adult JOs, no such expression was found for ato. Consistent with this finding, an adult-specific knock-down (KD) of ato did not have any significant effect on fly hearing (Supplementary Table 6). This does, however, not exclude the possibility that perturbing ato expression developmentally might affect the ear’s homeostatic resilience and lead to dysfunction later in life, as has been shown for Atoh1 in the mouse cochlea65.

The KD of amos, in contrast, produces an accelerated hearing loss phenotype that is characterised by a loss of power gain and tuning sharpness. Interestingly though, best frequencies of amos KD receivers do not move towards the passive system but instead show a small - but significant - move in the opposite direction, indicating a larger independence between fundamental parameters of Drosophila hearing than appreciated by current models17,66. amos KD also leads to a loss of nerve responses in high-threshold units of JO and a homeostatic reorganization of sensitive transducer channels, characterised by a slight decrease in single channel gating forces and a slight increase in channel number (Fig. 4d). Consistent with bioinformatical predictions, qPCR analyses of JOs of amos KD flies showed significantly reduced expression levels for the here newly described auditory dynein Dhc98D but no effects on the three auditory TRP channels tested (nompC, nan, iav).

Interestingly, all four master regulators are predicted to act upstream of phototransduction genes (Fig. 2b), including visual opsins, which have been previously linked to Drosophila auditory function28 and ciliary maintenance67 and are also upregulated during auditory ageing (Fig. 2a). This indicates a substantial regulatory overlap between the auditory and the visual system, which might not be restricted to Drosophila as a brief comparison with the respective mammalian transcriptomes suggests (see Supplementary Table 5 for details). 78% of the predicted regulators (29 human orthologues of 37 Drosophila TFs) were previously shown to be expressed in the human retina and associated with age-related macular degeneration (AMD)68. Shared homeostasis genes may well be a molecular substrate for auditory/visual co-morbidities (e.g. ARHL + AMD).

The human orthologues of 29 predicted TFs, finally, were found to be expressed in the adult human inner ear (see Supplementary Table 5 for details)69, including close orthologues of amos (ATOH8), Optix (SIX1, SIX2 and SIX4), and orthologues of wor (SNAI1, SNAI2, SNAI3). The human orthologue of Drosophila sox14 (SOX4) has also recently been identified in a GWAS of age-related hearing loss15. Down-regulation of sox14 in flies results in a hearing loss phenotype (see Supplementary Table 6). Most of the other predicted TFs, which showed functional relevance in our study are conserved, and expressed, in the human inner ear, e.g. aop (ETV5), ara (IRX1-3), lola (ZBTB20), pnr (GATA2, GATA3), run (RUNX1, RUNX2), ct (CUX1, CUX2), and Stat92E (STAT1-6); or in the mouse inner ear, onecut (Onecut3), Optix (Six1-6), Pph13 (Alx3), wor (Snai1, Snai2), amos (Atoh1, Neurod1, Neurod6).

These findings reinforce the narrative of a transcriptional homeostatic machinery, which is conserved between flies and humans and required to maintain not only hearing but also vision.

Our study has identified novel master regulators of auditory maintenance, some of which work as bidirectional homeostatic actuators within the fly’s auditory neurons. If the regulator’s upregulation, e.g., results in an improvement of a specific auditory function, then its downregulation leads to a worsening (amos), or vice versa (Optix).

It seems obvious that homeostatic mechanisms will not be restricted to the transcriptomic level but extend further to the auditory proteome. In fact, the prominence of age-variable heat-shock proteins and kinases in our own transcriptomic data clearly points to the relevance of post-translational, e.g. proteostatic, mechanisms. The vital role proteostasis plays in general ageing70 and hearing in particular71,72 is becoming increasingly recognised and also merits further exploration in the Drosophila ear.

Future studies will apply the powerful combination of transcriptome profiling and computational analyses, which has already contributed to advancing our knowledge of the complex regulatory networks underlying hearing and deafness73 and will also shed more light on the downstream targets of the here identified transcription factors and their specific roles in auditory homeostasis. Some key conclusions, however, can be drawn already. All four master regulators that emerged from our screen are evolutionary conserved; they either form key regulators of specific sensory (or neural) tissues or constitute paralogs of such regulators; their predicted (and in part validated) regulons, however, do not comprise of classic developmental genes (such as proliferation, apoptosis) but rather of known effector genes for specific auditory functions, e.g. ion channels and motor proteins. This suggests a scenario where developmental and homeostatic functions are divided between pairs (or groups) of paralogs. Examples for such pairs from our study would be ato/amos or ct/onecut. Sometimes, as is the case for the proneural master gene ato, the homeostatic roles seem to have been fully transferred to a paralog (amos). The 19th century recapitulation theory (or biogenetic law)74 proposed that ontogeny recapitulates phylogeny to explain the phenotypic similarities between early developmental stages of evolutionarily younger species (e.g. mammals) and more adult stages of evolutionarily older species (e.g. fish). In analogy, one might propose that an organ’s homeostatic maintenance (organostasis) partly recapitulates its development (organogenesis). The original biogenetic law has meanwhile been refined, and rewritten, as hourglass model of evolution, which posits that for every animal there is a specific phylotypic stage during which it most closely resembles other species75. This resemblance also extends to the molecular level: Expression patterns of key developmental genes are most conserved between species during this phylotypic (or also organotypic) phase76. Together with the reported high conversation of binding specificities between fly and human TF orthologues77, an hourglass model of sensory homeostasis might indeed be a valuable guide for the translational route from Drosophila ear to human cochlea. This could also have implications for the design of gene-therapeutic trials to reverse human hearing loss, which currently concentrate on key developmental genes - such as e.g. ATOH1. ATOH1’s ‘next of kin‘ – such as e.g. ATOH7, ATOH8 or NEUROD1 – might be worth having a look at.

Materials and Methods

Rearing conditions for auditory ageing

Unless otherwise specified, flies were raised on standard medium in incubators maintained at 25 °C and 60% relative humidity (RH), with a 12 hr:12 hr light:dark cycle. Virgin female and male flies were collected on the day of eclosion using CO2 sedation and allowed to age in separate vials at 25 °C for 1, 5, 10, 25, 50, 60 and 70 days – all biomechanical and electrophysiological experiments were conducted at room temperature (21 °C–22 °C). Adult-specific RNAi knock-down mutants (whose larvae and pupae were kept at 18 °C in order to repress the Gal4-mediated transcriptional activation via a Gal80ts repressor) were collected on the day of eclosion and transferred to 30 °C (for maximal activation of the Gal4/UAS expression system), 60% RH and kept at 12 hr:12 hr light:dark cycles for 2 weeks prior to the experiments. Flies were raised under conditions, which formed a near zero-noise environment for their particle velocity sensitive antennal receivers. Conditions included: (i) separate housing of virgin males and females at low densities (20-25 flies per vial), in (ii) environmentally controlled incubators, with (iii) regular transfer to fresh medium (twice a week) and at ambient sound levels below the hearing threshold. Antennal stimulation across the flies’ life course was thus occurring almost exclusively as a result of the animals’ own locomotion. As a result of the low density of their housing and the abundance of food no aggressive interactions were observed.

Life span measurements

Three independent cohorts of male Canton-S flies were set up in parallel. The density of flies per vial (25) was kept constant, the flies were transferred to a fresh medium every 3 days, and the number of dead flies was counted. The flies were kept at 60% RH and kept at a 12 hr:12 hr light:dark cycles for approx. 80 days. Rearing conditions were identical to the ones used for the auditory ageing experiments described above.

Fly stocks used

To assess the natural life course of hearing in Drosophila the following lines were used as wildtype references: Canton-S line (Bloomington), Canton-S (Goodwin lab), Canton-S (Kamikouchi lab), Oregon-R.

To probe the expression of predicted transcription factors the following lines used: Fly-TransgeneOme (fTRG) sGFP tagged lines from VDRC78 for amos, onecut and Optix (optix:GFP 318371/10042), wor-Gal4 (kindly provided by A. Carmena).

elav-Gal4; UAS-RFP-nls/+; Mi{PT-GFSTF.0}alphaTub85E[MI08426-GFSTF.0]/+ was used to monitor JO neurons across the flies’ lifespan.

y[1]w[*]; tub-Gal80ts; NP0761 was used for adult-specific downregulation (via RNAi knock-down) or upregulation (via overexpression) of target genes across all JO neurons.

RNAi lines were obtained from the Bloomington Drosophila Stock Centre (BDSC) and Vienna Drosophila Research Centre (VDRC). Attp2 and attp40 served as control lines for the TRIP collection and VDRC 6000 was used as control for the KK lines.

y[1] sc[*] v[1]; P{y[+t7.7] v[+t1.8]=TRiP.HMS01438}attP2 onecut RNAi

y[1] v[1]; P{y[+t7.7] v[+t1.8]=TRiP.JF02254}attP2 lola RNAi

y[1] v[1]; P{y[+t7.7] v[+t1.8]=TRiP.HM05094}attP2 srp RNAi

y[1] v[1]; P{y[+t7.7] v[+t1.8]=TRiP.JF02518}attP2 Rfx RNAi

y[1] sc[*] v[1]; P{y[+t7.7] v[+t1.8]=TRiP.HMS00924}attP2 ct RNAi

y[1] sc[*] v[1]; P{y[+t7.7] v[+t1.8]=TRiP.HMS01186}attP2/TM3, Sb[1] run RNAi

y[1] sc[*] v[1]; P{y[+t7.7] v[+t1.8]=TRiP.HMS01430}attP2 ato RNAi

y[1] sc[*] v[1]; P{y[+t7.7] v[+t1.8]=TRiP.HMS01256}attP2 aop RNAi

y[1] v[1]; P{y[+t7.7] v[+t1.8]=TRiP.HMC03993}attP2 Optix RNAi

y[1] sc[*] v[1]; P{y[+t7.7] v[+t1.8]=TRiP.HMC04197}attP40 Tbp RNAi

y[1] sc[*] v[1]; P{y[+t7.7] v[+t1.8]=TRiP.HMS01082}attP2 pnr RNAi

y[1] v[1]; P{y[+t7.7] v[+t1.8]=TRiP.HMC03988}attP2 gl RNAi

y[1] sc[*] v[1]; P{y[+t7.7] v[+t1.8]=TRiP.HMS00103}attP2 sox14 RNAi

y[1] sc[*] v[1]; P{y[+t7.7] v[+t1.8]=TRiP.HMC05094}attP40 amos RNAi

y[1] v[1]; P{y[+t7.7] v[+t1.8]=TRiP.HMS00035}attP2 Stat92E RNAi

y[1] v[1]; P{y[+t7.7] v[+t1.8]=TRiP.JF02233}attP2 Aef1 RNAi

VDRC 110594 KK line Pph13 RNAi

VDRC 105362 KK line wor RNAi

VDRC 101903 KK line ara RNAi

y[1]w[*]; P{UAS-Optix.S}1

w[*]; P{UAS-amos.G}5

w[*]; P{UAS-ato.J}8/TM3, Sb1

w[*]; P{UAS-wor} [kindly provided by J.Knoblich]

y[1] sc[*] v[1] sev[21]; P{y[+t7.7] v[+t1.8]=TRiP.HMC06494}attP40 Dhc98D RNAi

Immunostainings of JO

To probe the expression of predicted transcription factors, the following lines were used: Fly-TransgeneOme (fTRG) sGFP tagged lines from VDRC78 for amos, onecut and Optix (optix:GFP 318371/10042), wor-Gal4 (kindly provided by A. Carmena).

Fixation and immunostainings followed standard procedures. Briefly, 10 days old adult female heads were dissected in PBS, fixed with a 4% formaldehyde solution (in PBT) for one hour while rotating at room temperature (RT); three heads were placed exposing the antennae into silicon blocks filled previously with hot gelatin-albumin mixture. Silicone blocks were then quickly cooled down at 4 °C for 10 minutes and incubated with 6% formaldehyde solution overnight at 4 °C. Thereafter, silicone blocks were extracted and incubated further with Methanol for 10 min at RT, before being washed with PBS for 30 min at RT. 30 µm vibratome sections were cut using a vibratome (Ci 5100mz, Campden Instruments) and antennae sections collected in PBT (PBS with 0.3% Triton X-100) and afterwards washed three times for 15 min at RT. After blocking for 1 hr at RT (blocking solution: PBS with 1% Triton X-100, 2% BSA, 5% normal goat serum), samples were incubated with primary antibodies in blocking solution overnight at 4 °C, then washed again three times in PBT and incubated with secondary antibodies diluted in blocking solution for 2 hr at RT. Samples were then washed again three times in PBT and, finally, briefly washed in PBS before mounting. Primary antibodies used in this study are:

Rb anti-GFP 1:1000 (Life Technologies), Rat anti-elav 1:250 (Hybridoma Bank), Goat anti-HRP::Cy3 1:500 (Jackson ImmunoResearch). Secondary antibodies conjugated with Alexa 488, and Alexa 633 (Life Technologies) were used at 1:500. All samples were mounted in Dabco (Molecular Probes, H-1200). Images were acquired with a LSM 510 Zeiss confocal microscope with a Plan-Neofluar 40×/1.3 Oil objective. Z-stacks (optical slice thickness: 1μm) were taken to image throughout Johnston’s organ (JO). Images were assembled and analysed in ImageJ (Fiji).

Immunostainings of pharate adult JOs

The RNAi line for onecut was crossed to iav-Gal4, iav::GFP. Crosses were kept at 18 °C until the 3rd instar larval stage and then shifted to 25 °C. The antennae of pharate adult flies (post-metamorphosis but pre-eclosion) were fixed in 3.7% formaldehyde for 30 min and blocked for>2 h in 3% BSA at RT. Primary antibodies were added for 48 h and secondary antibodies overnight at 4 °C. Alexa568-conjugated phalloidin (Molecular Probes, 1:2000) was added for 45 min at RT following incubation with secondary antibody. Rb anti-GFP (Invitrogen), anti-RbAlexa488 (Molecular Probes) were used at 1:500.

Neuron counts

Flies of genotype elav-Gal4; UAS-RFP-nls/+; Mi{PT-GFSTF.0}alphaTub85E[MI08426-GFSTF.0]/+ were aged at 25 °C. Fly antennae of day1, day5, day25 and day 50 flies were dissected in PBS, such that left and right antennae remained attached to the cuticle, and that the third antennal segment and the associated arista remained intact. Antennae were then briefly fixed for 10 minutes in 4% formaldehyde in PBS, washed three times in PBT and finally mounted in glycerol. Fly JO-s were imaged with an LSM 510 Zeiss confocal microscope with a Plan-Neofluar 40×/1.3 Oil objective. Z-stacks (optical slice thickness: 1μm, 80 slices in total) were taken to image throughout Johnston’s organ (JO). Images were processed and unspecific background removed using the FluoRender programme. Single Z-stacks were processed in ImageJ. The Eve programme (based on the algorithm from Shimada et al. 2005 and kindly provided by Kei Ito)79 was used to count neurons automatically (XY:Z ratio was set depending on the number of the stacks), neuron radius was set to 4 and Bending 1 at 300 cells was used as a cut-off. Processed images were saved as new files (including cell count information) and result files were produced. Number of cells was corrected manually by using the ImageJ cell counter plugin.

RNA sequencing

Virgin male and female Canton-S flies of different ages (days 1, 5, 10, 25, and 50) were anesthetised on ice, their second antennal segments dissected and collected in Lysis Buffer (containing 1% β-mercaptoethanol, as provided in the Qiagen RNeasy Mini Kit). As soon as dissections were completed for a given time point, samples were frozen at −80 °C. When enough samples were collected, RNA was extracted according to the Qiagen RNeasy Mini Kit protocol.

Reverse transcription and pre-amplification were carried out with the SMART-Seq v4 Ultra Low Input RNA Kit for Sequencing (Clontech). All samples were quality controlled and cDNA concentrations measured with an Agilent BioAnalyzer 2100. Sample libraries were prepared with a Nextera XT DNA Library Preparation kit (Illumina). Thereafter, paired-end 75 bp reads were sequenced on an Illumina NextSeq 500 platform.

The RNAseqfastq files were aligned in the Partek Flow software to the most recent version of the Drosophila genome (dm6) obtained from the Berkeley Drosophila Genome Project at UCSC.

In order to generate raw sequence counts, .bam files created in Partek software were processed in HTSeq These counts were then used in DESeq2 in R/Bioconductor to measure differential expression across genes and for conducting ANOVA statistical analyses of each comparison. Further data filtering took place to reduce the maximum false discovery rate (FDR) to 10% limiting the expression fold change threshold to ±1.5×.

Quantitative PCR (qPCR)

Flies of different genotypes were collected and frozen immediately with liquid nitrogen and then kept at −80 °C. After 50 flies were collected they were vortexed and second antennal segments were collected (100 antennae) in Lysis Buffer containing 1% β-mercaptoethanol (as part of the Qiagen RNeasy Mini Kit). In accordance with the Qiagen RNeasy Mini Kit protocol, RNA was extracted immediately and RNA samples were then kept at −80 °C.

Reverse transcription was carried out with the High Capacity RNA to cDNA kit (Applied Biosystems) following the manufacturer’s protocol.

In order to proceed to pre-amplification with TaqMan PreAmp Master Mix Kit, a “pooled assay” of Taqman primers was prepared (containing probes for the target genes of interest, i.e. nompC, nan, iav, Dhc98D). TaqMan probes of interest were mixed together and diluted 1:100 in TE buffer. The pre-amplification procedure followed the manufacturer’s protocol. The pre-amplified cDNA was diluted 1:20 in RNAse and DNAse-free water and the qPCR was performed in the immediate aftermath. qPCR assays were run on a Step One Plus ABI machine. Prior to the reaction, the 96 well plate set up was designed with help of the Step One Plus software. Three negative controls were run per target as well as three replicates for each sample and each target. SdhA was chosen as endogenous control as one of the housekeeping genes that has the most stable expression at different ages80.Reactions were prepared according to the TaqMan Gene Expression Assay protocol.

Cycle threshold (Ct) values were extracted from the Step One Plus Software data analysis. The ΔΔCt and relative q

$${\Delta }Ct=(C{t}_{gene}\times control-C{t}_{endogenouscontrol})$$
$$\varDelta \varDelta Ct=\,\varDelta Ct-(C{t}_{gene}\times knockdown-C{t}_{endogenouscontrol})$$
$$RQ={2}^{-\varDelta \varDelta Ct}$$

The three RQ values were averaged for each biological replicate and standard deviations generated in Excel. At least three biological replicates were performed for each experiment. Statistical were performed in SigmaPlot.

Bioinformatical analysis in iRegulon

The iRegulon plug-in41 was used in the Cytoscape software to predict transcription factors/regulators based on their binding motifs. A list of genes of interest was submitted and predicted transcription factors were then selected according to their normalised enrichment scores (NES) for a particular motif, or group of motifs, within the list originally submitted to iRegulon.

Gene ontology analysis - GORILLA

The online interface GOrilla (Gene Ontology enRIchment anaLysis and visuaLizAtion tool) was used to classify genes of interest according to their gene ontology37,38

Functional classifications were generated for biological processes and molecular functions. Enrichment scores were calculated:

$${\rm{Enrichment}}=(b/{\rm{n}})/(B/N),$$

where b is the number of genes in the intersection, n the number of genes in the target set, B the total number of genes associated with a specific GO term and N the total number of genes.

Preparation of gene lists for submission to iRegulon and transcription factor (TF) selection

Submission round I

The identified 5,855 age-variable genes were submitted to the Gene Ontology enRIchment anaLysis and visualization (GOrilla) tool. Gene sets from four hearing-relevant gene ontological categories ([i] trafficking genes, [ii] structural genes, [iii] dynein motor proteins and [iv] receptors, see Suppl. Figure 2) were then submitted to iRegulon to predict their upstream regulatory genes (TFs) based on binding motif enrichment scores (cut-off: threshold 2.5, Rank threshold: 5,000). This generated a first list of candidate TFs.

Submission round II

The most highly expressed age-variable genes (>10,000 reads) were submitted to iRegulon (same cut-off thresholds as above). This generated a second list of candidate TFs.

Submission round III

Genes showing the greatest age-variability (down- or up-regulated by at least 4-times in at least one age comparison) were submitted to iRegulon (same cut-off thresholds as above). This generated a third list of candidate TFs.

In a final step, all candidate TFs (from I-III above) were filtered further to choose those subjected to functional testing: (i) suitable transcription factors had to show expression in JO, i.e. they had to be part of the 16,243 genes identified in our RNA-Seq (see Suppl Table 2). This brought the total number of TFs to 37 (see Suppl. Table 5); (ii) a random (~50%) selection of these TFs (19 in total) was then chosen for functional biomechanical tests (fluctuation analyses) in RNAi knockdown lines. The four TFs showing the strongest phenotypes (Onecut, Amos, Optix, Worniu) were then chosen for in-depth functional characterisation.

JO functional analyses

For all analyses of JO function, flies were mounted as described previously16. Briefly, flies were attached, ventrum-down, to the head of a Teflon rod using blue light-cured dental glue. The second segment of the antenna under investigation was glued down to prevent non-auditory background movements. The antenna not under investigation was glued down in its entirety, thereby completely abolishing any sound-induced motion and interference with the contralateral recordings. An active vibration isolation table (model 63-564; TMC, USA) was used. After mounting, flies were oriented such that the antennal arista was perpendicular to the beam of a laser Vibrometer (PSV-400; Polytec, Germany) and free fluctuation recordings could be taken. To allow for ultrafast, contact-free, non-loading stimulation, electrostatic actuation (EA) was used. EA is conducted via two external actuators positioned close to the arista (for details see Albert et al.16, and Effertz et al.53).Two electrodes were inserted into the fly – a charging electrode was placed into the thorax so that the animal’s electrostatic potential could be raised to −20 V against ground, and a recording electrode for measuring mechanically evoked compound action potentials (CAPs) was introduced close to the base of the antenna under investigation. The charging electrode also served as reference electrode for the CAP recordings.

Arista displacements were measured at the arista’s tip using a PSV-400 LDV with an OFV-70 close up unit (70 mm focal length) and a DD-500 displacement decoder. The displacement output was digitized at a rate of 100 kHz using a CED Power 1401 mk II A/D converter and loaded into the Spike 2 software (both Cambridge Electronic Design Ltd., Cambridge, England). Free (i.e. unstimulated) fluctuations of the arista were recorded both before and after the experiment to monitor the physiological integrity of the antennal ear. Free fluctuations were then analysed in SigmaPlot (Systat Software, Inc), where simple harmonic oscillator models were fitted to the velocity data as previously described18,23 (see also Supplementary Fig. 6). Median fits (calculated from the median values of individual fits) are shown as line plots (Figs. 1c, 4a and 5b; Supplementary Figs. 5 and 6b). Only those flies, which maintained a stable antennal function throughout the experiment (maximally allowed change of best frequencies: 20%) were analysed.

Approximate equivalence of hearing parameters between Drosophila and humans: analyses of the fly’s auditory mechanics (free fluctuation and gating compliance analyses) probe for hearing loss that originates within the chordotonal transducer sites proper (human equivalent: stereociliary bundles of hair cells). Calculated power gain values quantify hearing sensitivity; the maximal gain of the fly’s auditory amplifier is ~20–30 dB (the gain of its functional equivalent, the human cochlear amplifier, is ~50–60 dB). CAP responses roughly correspond to human ABR measurements. Together, the used set of measurements allows for allocating the likely cause of the observed hearing impairments (loss of transduction, loss of amplification or neuropathy). Please note that Drosophila chordotonal neurons – in contrast to human hair cells - are primary neurons, which directly send axon potentials to the brain.

Tests of sound-evoked behaviour

Drosophila melanogaster males increase locomotor activity in response to a playback of courtship songs31. We exploited this phenomenon to test hearing across the Drosophila life course. To conduct measurements, flies were housed in 5 × 65 mm Pyrex glass tubes. One end of the tube was sealed with an acoustically transparent mesh, the other end contained food consisting of 5% sucrose and 2% agar medium covering ~¼ of the tube. Glass tubes were then loaded into high-resolution Drosophila activity monitors (MB5; Trikinetics, Walham, USA). MB5 monitors harbour 17 independent infrared (IR) beams bisecting each tube at 3 mm intervals, allowing for a high-fidelity recording of the flies’ activity. Detectors were set to count all beam breaks occurring within one minute for the duration of each experiment. Activity counts were registered independently at each beam position within a tube; all beam breaks, irrespective of beam position, were then pooled. This procedure allowed for calculating the total activity of all flies in that tube. To maximise data collection, three MB5 monitors were stacked together forming a grid allowing to record from 36 tubes (totalling 108 flies) simultaneously over the course of a single experiment. The MB5 activity monitors were placed centrally in front of a 381 mm wide bass speaker (Eminence Delta 15, 400 W, 8 ohm) with the tubes’ acoustically transparent mesh facing the speaker at a distance of ~60 mm from the speaker membrane. The speaker was connected to an amplifier (Prosound 1600W). To avoid interference from non-air-borne vibrations, the MB5 monitors – but not the speaker - were placed on a vibration isolation table. Sound stimuli were adjusted to reach peak amplitudes of 90 dB SPL at the middle of the monitor tubes. Courtship stimuli played at these intensities are known to elicit reproducible behavioural responses in males81. The sound stimulus (played, and controlled from the Spike2 software) consisted of a ‘master pulse’ that was repeated to form 2 s long trains with 40 ms interpulse intervals (IPIs). The master pulse was generated by averaging previously recorded original courtship song pulses (~1000 pulses from 10 Drosophila melanogaster males). Each pulse train was followed by a 2 s long silence; this elementary kernel was played continuously for 15 minutes at the beginning of every hour. The 15 min of sound stimulation were played in loop with 45 min of silence for an entire circadian day (24 h at a 12-hour light, 12-hour dark cycle). Responses for each hour were then collapsed into a single median response to cancel out any circadian variations of responsiveness.

Activity displayed during stimulus presentation was determined by the sum of all activity displayed during the first 15 minutes of every hour (i.e. during the phase of sound stimulation) and averaged over the whole experimental day. Baseline activity was determined by the sum of all activity displayed during the last 15 minutes of every hour (i.e. during the silent phase directly preceding the next stimulus phase) and also averaged over the whole experimental day.

The room, in which the recordings took place was held at a constant 25 °C temperature (@ ~40% RH) and followed a 12-hour light, 12-hour dark cycle, which was kept consistent with the flies’ entrainment regime prior to experiment start. Exposure to courtship sound is known to induce male flies to also produce mating songs. To prevent these stimulus-induced mating songs from interfering with the sound stimulus, experimental flies were anaesthetized using CO2 and their wings clipped 2-4 days prior to the initiation of the experiment. At least 2/3 of the wing was removed using microdissection scissors. After allowing time for healing post procedure, the flies were again CO2-anesthetized and transferred into the glass tubes before being placed into the MB5 monitors. For each experiment, flies were exposed to the sound stimulus as soon as they were placed into the monitors; however, only data recorded from the first light transition on was used for analysis. This allowed flies to have ~12 hr to adapt to the stimulus, the new environment and to recover from after-effects of CO2 exposure. After this equilibration stage, data was collected for 48 hours.

Data availability

The datasets generated and analysed during the current study are available in the the Gene Expression Omnibus (GEO) of the National Center for Biotechnology Information (NCBI); accession code: GSE148023 https://www.ncbi.nlm.nih.gov/geo/query/acc.cgi?acc=GSE148023.

References

  1. 1.

    WHO. WHO Deafness and Hearing, http://www.who.int/news-room/fact-sheets/detail/deafness-and-hearing-loss (2018).

  2. 2.

    Gates, G. A. & Mills, J. H. Presbycusis. Lancet 366, 1111–1120, https://doi.org/10.1016/S0140-6736(05)67423-5 (2005).

    Article  PubMed  Google Scholar 

  3. 3.

    Christensen, K., Frederiksen, H. & Hoffman, H. J. Genetic and environmental influences on self-reported reduced hearing in the old and oldest old. J Am Geriatr Soc 49, 1512–1517, https://doi.org/10.1046/j.1532-5415.2001.4911245.x (2001).

    CAS  Article  PubMed  Google Scholar 

  4. 4.

    Yamasoba, T. et al. Current concepts in age-related hearing loss: Epidemiology and mechanistic pathways. Hearing Research 303, 30–38, https://doi.org/10.1016/j.heares.2013.01.021 (2013).

    CAS  Article  PubMed  PubMed Central  Google Scholar 

  5. 5.

    Someya, S. et al. Age-related hearing loss in C57BL/6J mice is mediated by Bak-dependent mitochondrial apoptosis. Proceedings of the National Academy of Sciences of the United States of America 106, 19432–19437, https://doi.org/10.1073/pnas.0908786106 (2009).

    ADS  Article  PubMed  PubMed Central  Google Scholar 

  6. 6.

    Johnson, K. R., Erway, L. C., Cook, S. A., Willott, J. F. & Zheng, Q. Y. A major gene affecting age-related hearing loss in C57BL/6J mice. Hearing Research 114, 83–92, https://doi.org/10.1016/S0378-5955(97)00155-X (1997).

    CAS  Article  PubMed  Google Scholar 

  7. 7.

    Johnson, K. R., Zheng, Q. Y. & Erway, L. C. A Major Gene Affecting Age-Related Hearing Loss Is Common to at Least Ten Inbred Strains of Mice. Genomics 70, 171–180, https://doi.org/10.1006/geno.2000.6377 (2000).

    CAS  Article  PubMed  Google Scholar 

  8. 8.

    Johnson, K. R. et al. Separate and combined effects of Sod1 and Cdh23 mutations on age-related hearing loss and cochlear pathology in C57BL/6J mice. Hearing research 268, 85–92, https://doi.org/10.1016/j.heares.2010.05.002 (2010).

    CAS  Article  PubMed  PubMed Central  Google Scholar 

  9. 9.

    Avraham, K. B. et al. The mouse Snell’s waltzer deafness gene encodes an unconventional myosin required for structural integrity of inner ear hair cells. Nature genetics 11, 369–375, https://doi.org/10.1038/ng1295-369 (1995).

    CAS  Article  PubMed  Google Scholar 

  10. 10.

    Gibson, F. et al. A type VII myosin encoded by the mouse deafness gene shaker-1. Nature 374, 62, https://doi.org/10.1038/374062a0 (1995).

    ADS  CAS  Article  PubMed  Google Scholar 

  11. 11.

    Someya, S. et al. Sirt3 Mediates Reduction of Oxidative Damage and Prevention of Age-Related Hearing Loss under Caloric Restriction. Cell 143, 802–812, https://doi.org/10.1016/j.cell.2010.10.002 (2010).

    CAS  Article  PubMed  PubMed Central  Google Scholar 

  12. 12.

    Bowl, M. R. et al. A large scale hearing loss screen reveals an extensive unexplored genetic landscape for auditory dysfunction. Nature Communications 8, 886, https://doi.org/10.1038/s41467-017-00595-4 (2017).

    ADS  CAS  Article  PubMed  PubMed Central  Google Scholar 

  13. 13.

    Ingham, N. J. et al. Mouse screen reveals multiple new genes underlying mouse and human hearing loss. Plos Biology 17, e3000194, https://doi.org/10.1371/journal.pbio.3000194 (2019).

    CAS  Article  PubMed  PubMed Central  Google Scholar 

  14. 14.

    Potter, P. K. et al. Novel gene function revealed by mouse mutagenesis screens for models of age-related disease. Nature Communications 7, 13, https://doi.org/10.1038/ncomms12444 (2016).

    CAS  Article  Google Scholar 

  15. 15.

    Wells, H. R. R. et al. GWAS Identifies 44 Independent Associated Genomic Loci for Self-Reported Adult Hearing Difficulty in UK Biobank. Am J Hum Genet 105, 788–802, https://doi.org/10.1016/j.ajhg.2019.09.008 (2019).

    CAS  Article  PubMed  PubMed Central  Google Scholar 

  16. 16.

    Albert, J. T., Nadrowski, B. & Göpfert, M. C. Mechanical signatures of transducer gating in the Drosophila ear. Curr Biol 17, 1000–1006, https://doi.org/10.1016/j.cub.2007.05.004 (2007).

    CAS  Article  PubMed  Google Scholar 

  17. 17.

    Nadrowski, B., Albert, J. T. & Gopfert, M. C. Transducer-based force generation explains active process in Drosophila hearing. Current Biology 18, 1365–1372, https://doi.org/10.1016/j.cub.2008.07.095 (2008).

    CAS  Article  PubMed  Google Scholar 

  18. 18.

    Göpfert, M. C., Humphris, A. D., Albert, J. T., Robert, D. & Hendrich, O. Power gain exhibited by motile mechanosensory neurons in Drosophila ears. Proceedings of the National Academy of Sciences of the United States of America 102, 325–330, https://doi.org/10.1073/pnas.0405741102 (2005).

    ADS  CAS  Article  PubMed  Google Scholar 

  19. 19.

    Kamikouchi, A. et al. The neural basis of Drosophila gravity-sensing and hearing. Nature 458, 165, https://doi.org/10.1038/nature07810 (2009).

    ADS  CAS  Article  PubMed  Google Scholar 

  20. 20.

    Jarman, A. P., Grau, Y., Jan, L. Y. & Jan, Y. N. atonal is a proneural gene that directs chordotonal organ formation in the Drosophila peripheral nervous system. Cell 73, 1307–1321 (1993).

    CAS  Article  Google Scholar 

  21. 21.

    Bermingham, N. A. et al. Math1: an essential gene for the generation of inner ear hair cells. Science 284, 1837–1841 (1999).

    CAS  Article  Google Scholar 

  22. 22.

    Wang, V. Y., Hassan, B. A., Bellen, H. J. & Zoghbi, H. Y. Drosophila atonal fully rescues the phenotype of Math1 null mice: New functions evolve in new cellular contexts. Current Biology 12, 1611–1616, https://doi.org/10.1016/S0960-9822(02)01144-2 (2002).

    CAS  Article  PubMed  Google Scholar 

  23. 23.

    Weinberger, S. et al. Evolutionary changes in transcription factor coding sequence quantitatively alter sensory organ development and function. eLife 6, e26402, https://doi.org/10.7554/eLife.26402 (2017).

    Article  PubMed  PubMed Central  Google Scholar 

  24. 24.

    Li, T. C., Bellen, H. J. & Groves, A. K. Using Drosophila to study mechanisms of hereditary hearing loss. Dis. Model. Mech 11, 16, https://doi.org/10.1242/dmm.031492 (2018).

    CAS  Article  Google Scholar 

  25. 25.

    Kavlie, R. G. et al. Prestin is an anion transporter dispensable for mechanical feedback amplification in Drosophila hearing. J. Comp. Physiol. A -Neuroethol. Sens. Neural Behav. Physiol 201, 51–60, https://doi.org/10.1007/s00359-014-0960-9 (2015).

    CAS  Article  PubMed  Google Scholar 

  26. 26.

    Kamikouchi, A., Albert, J. T. & Gopfert, M. C. Mechanical feedback amplification in Drosophila hearing is independent of synaptic transmission. European Journal of Neuroscience 31, 697–703, https://doi.org/10.1111/j.1460-9568.2010.07099.x (2010).

    Article  PubMed  Google Scholar 

  27. 27.

    Karak, S. et al. Diverse Roles of Axonemal Dyneins in Drosophila Auditory Neuron Function and Mechanical Amplification in Hearing. Scientific Reports 5, https://doi.org/10.1038/srep17085 (2015).

  28. 28.

    Senthilan, P. R. et al. Drosophila auditory organ genes and genetic hearing defects. Cell 150, 1042–1054, https://doi.org/10.1016/j.cell.2012.06.043 (2012).

    CAS  Article  PubMed  Google Scholar 

  29. 29.

    Kavlie, R. G. & Albert, J. T. Chordotonal organs. Current Biology 23, R334–R335 (2013).

    CAS  Article  Google Scholar 

  30. 30.

    Kamikouchi, A., Shimada, T. & Ito, K. Comprehensive classification of the auditory sensory projections in the brain of the fruit fly Drosophila melanogaster. J Comp Neurol 499, 317–356, https://doi.org/10.1002/cne.21075 (2006).

    Article  PubMed  Google Scholar 

  31. 31.

    von Schilcher, F. The role of auditory stimuli in the courtship of Drosophila melanogaster. Animal Behaviour 24, 18–26 (1976).

    Article  Google Scholar 

  32. 32.

    Ruhmann, H., Koppik, M., Wolfner, M. F. & Fricke, C. The impact of ageing on male reproductive success in Drosophila melanogaster. Experimental Gerontology 103, 1–10, https://doi.org/10.1016/j.exger.2017.12.013 (2018).

    Article  PubMed  Google Scholar 

  33. 33.

    Prathibha, M., Krishna, M. S. & Jayaramu, S. C. Male age influence on male reproductive success in Drosophila ananassae (Diptera: Drosophilidae). Ital. J. Zoolog 78, 168–173, https://doi.org/10.1080/11250003.2011.564214 (2011).

    Article  Google Scholar 

  34. 34.

    Albert, JoergT. & Kozlov, Andrei S. Comparative Aspects of Hearing in Vertebrates and Insects with Antennal Ears. Current Biology 26, R1050–R1061, https://doi.org/10.1016/j.cub.2016.09.017 (2016).

    CAS  Article  PubMed  Google Scholar 

  35. 35.

    Markin, V. S. & Hudspeth, A. J. Gating-Spring Models of Mechanoelectrical Transduction by Hair Cells of the Internal Ear. Annual Review of Biophysics and Biomolecular Structure 24, 59–83, https://doi.org/10.1146/annurev.bb.24.060195.000423 (1995).

    CAS  Article  PubMed  Google Scholar 

  36. 36.

    Albert, J. T., Nadrowski, B. & Göpfert, M. C. Drosophila mechanotransduction - Linking proteins and functions. Fly 1, 238–241 (2007).

    Article  Google Scholar 

  37. 37.

    Eden, E., Lipson, D., Yogev, S. & Yakhini, Z. Discovering motifs in ranked lists of DNA sequences. Plos Computational Biology 3, 508–522, https://doi.org/10.1371/journal.pcbi.0030039 (2007).

    MathSciNet  CAS  Article  Google Scholar 

  38. 38.

    Eden, E., Navon, R., Steinfeld, I., Lipson, D. & Yakhini, Z. GOrilla: a tool for discovery and visualization of enriched GO terms in ranked gene lists. Bmc Bioinformatics 10, https://doi.org/10.1186/1471-2105-10-48 (2009).

  39. 39.

    Roy, M., Sivan-Loukianova, E. & Eberl, D. F. Cell-type–specific roles of Na+/K+ ATPase subunits in Drosophila auditory mechanosensation. Proceedings of the National Academy of Sciences 110, 181–186, https://doi.org/10.1073/pnas.1208866110 (2013).

    ADS  Article  Google Scholar 

  40. 40.

    Christie, K. W. et al. Physiological, anatomical, and behavioral changes after acoustic trauma in Drosophila melanogaster. Proceedings of the National Academy of Sciences of the United States of America 110, 15449–15454, https://doi.org/10.1073/pnas.1307294110 (2013).

    ADS  Article  PubMed  PubMed Central  Google Scholar 

  41. 41.

    Janky, R. s. et al. iRegulon: From a Gene List to a Gene Regulatory Network Using Large Motif and Track Collections. Plos Computational Biology 10, e1003731, https://doi.org/10.1371/journal.pcbi.1003731 (2014).

    CAS  Article  PubMed  PubMed Central  Google Scholar 

  42. 42.

    Dubruille, R. et al. Drosophila regulatory factor X is necessary for ciliated sensory neuron differentiation. Development 129, 5487–5498, https://doi.org/10.1242/dev.00148 (2002).

    CAS  Article  PubMed  Google Scholar 

  43. 43.

    Ebacher, D. J. S., Todi, S. V., Eberl, D. F. & Falk, G. E. B. cut mutant Drosophila auditory organs differentiate abnormally and degenerate. Fly 1, 86–94, https://doi.org/10.4161/fly.4242 (2007).

    Article  PubMed  PubMed Central  Google Scholar 

  44. 44.

    Kim, J. et al. A TRPV family ion channel required for hearing in Drosophila. Nature 424, 81–84, https://doi.org/10.1038/nature01733 (2003).

    ADS  CAS  Article  PubMed  Google Scholar 

  45. 45.

    Gong, Z. et al. Two Interdependent TRPV Channel Subunits, Inactive and Nanchung, Mediate Hearing in Drosophila. The Journal of Neuroscience 24, 9059 (2004).

    CAS  Article  Google Scholar 

  46. 46.

    Effertz, T., Wiek, R., Gopfert, M. C. & NompC, T. R. P. Channel Is Essential for Drosophila Sound Receptor Function. Current Biology 21, 592–597, https://doi.org/10.1016/j.cub.2011.02.048 (2011).

    CAS  Article  PubMed  Google Scholar 

  47. 47.

    Kirkwood, T. B. L. Evolution of Aging. Nature 270, 301–304, https://doi.org/10.1038/270301a0 (1977).

    ADS  CAS  Article  PubMed  Google Scholar 

  48. 48.

    Gems, D. & Partridge, L. In Annual Review of Physiology, Vol 75 Vol. 75 Annual Review of Physiology (ed. D. Julius) 621–644 (Annual Reviews, 2013).

  49. 49.

    Nguyen, D. N. T., Rohrbaugh, M. & Lai, Z.-C. The Drosophila homolog of Onecut homeodomain proteins is a neural-specific transcriptional activator with a potential role in regulating neural differentiation. Mechanisms of Development 97, 57–72, https://doi.org/10.1016/S0925-4773(00)00431-7 (2000).

    CAS  Article  PubMed  Google Scholar 

  50. 50.

    Wu, F., Sapkota, D., Li, R. & Mu, X. Onecut 1 and Onecut 2 are potential regulators of mouse retinal development. The Journal of Comparative Neurology 520, 952–969, https://doi.org/10.1002/cne.22741 (2012).

    CAS  Article  PubMed  PubMed Central  Google Scholar 

  51. 51.

    Nesterov, A. et al. TRP Channels in Insect Stretch Receptors as Insecticide Targets. Neuron 86, 665–671, https://doi.org/10.1016/j.neuron.2015.04.001 (2015).

    CAS  Article  PubMed  Google Scholar 

  52. 52.

    Lehnert, B. P., Baker, A. E., Gaudry, Q., Chiang, A.-S. & Wilson, R. I. Distinct Roles of TRP Channels in Auditory Transduction and Amplification in Drosophila. Neuron 77, 115–128, https://doi.org/10.1016/j.neuron.2012.11.030 (2013).

    CAS  Article  PubMed  Google Scholar 

  53. 53.

    Effertz, T., Nadrowski, B., Piepenbrock, D., Albert, J. T. & Göpfert, M. C. Direct gating and mechanical integrity of Drosophila auditory transducers require TRPN1. Nature Neuroscience 15, 1198–1200, https://doi.org/10.1038/nn.3175 (2012).

    CAS  Article  PubMed  Google Scholar 

  54. 54.

    Gopfert, M. C., Albert, J. T., Nadrowski, B. & Kamikouchi, A. Specification of auditory sensitivity by Drosophila TRP channels. Nature Neuroscience 9, 999–1000, https://doi.org/10.1038/nn1735 (2006).

    CAS  Article  PubMed  Google Scholar 

  55. 55.

    Yan, Z. et al. Drosophila NOMPC is a mechanotransduction channel subunit for gentle-touch sensation. Nature 493, 221–225, http://www.nature.com/nature/journal/v493/n7431/abs/nature11685.html#supplementary-information (2013).

  56. 56.

    Zhang, W. et al. Ankyrin Repeats Convey Force to Gate the NOMPC Mechanotransduction Channel. Cell 162, 1391–1403, https://doi.org/10.1016/j.cell.2015.08.024 (2015).

    CAS  Article  PubMed  PubMed Central  Google Scholar 

  57. 57.

    Lai, S.-L., Miller, Michael R., Robinson, Kristin J. & Doe, Chris Q. The Snail Family Member Worniu Is Continuously Required in Neuroblasts to Prevent Elav-Induced Premature Differentiation. Developmental Cell 23, 849–857, https://doi.org/10.1016/j.devcel.2012.09.007.

  58. 58.

    Seimiya, M. & Gehring, W. J. The Drosophila homeobox gene optix is capable of inducing ectopic eyes by an eyeless-independent mechanism. Development 127, 1879 (2000).

    CAS  Google Scholar 

  59. 59.

    Jarman, A. P., Sun, Y., Jan, L. Y. & Jan, Y. N. Role of the proneural gene, atonal, in formation of Drosophila chordotonal organs and photoreceptors. Development 121, 2019–2030 (1995).

    CAS  PubMed  Google Scholar 

  60. 60.

    Jarman, A. P., Grell, E. H., Ackerman, L., Jan, L. Y. & Jan, Y. N. Atonal is the proneural gene for Drosophila photoreceptors. Nature 369, 398–400, https://doi.org/10.1038/369398a0 (1994).

    ADS  CAS  Article  PubMed  Google Scholar 

  61. 61.

    Gupta, B. P. & Rodrigues, V. Atonal is a proneural gene for a subset of olfactory sense organs in Drosophila. Genes to cells: devoted to molecular & cellular mechanisms 2, 225–233 (1997).

    CAS  Article  Google Scholar 

  62. 62.

    Goulding, S. E., zur Lage, P. & Jarman, A. P. amos, a proneural gene for Drosophila olfactory sense organs that is regulated by lozenge. Neuron 25, 69–78 (2000).

    CAS  Article  Google Scholar 

  63. 63.

    Huang, M. L., Hsu, C. H. & Chien, C. T. The proneural gene amos promotes multiple dendritic neuron formation in the Drosophila peripheral nervous system. Neuron 25, 57–67 (2000).

    Article  Google Scholar 

  64. 64.

    Maung, S. M. & Jarman, A. P. Functional distinctness of closely related transcription factors: a comparison of the Atonal and Amos proneural factors. Mech Dev 124, 647–656, https://doi.org/10.1016/j.mod.2007.07.006 (2007).

    CAS  Article  PubMed  PubMed Central  Google Scholar 

  65. 65.

    Xie, W. R. et al. An Atoh1-S193A Phospho-Mutant Allele Causes Hearing Deficits and Motor Impairment. J Neurosci 37, 8583–8594, https://doi.org/10.1523/jneurosci.0295-17.2017 (2017).

    CAS  Article  PubMed  PubMed Central  Google Scholar 

  66. 66.

    Nadrowski, B. & Göpfert, M. C. Level-dependent auditory tuning: Transducer-based active processes in hearing and best-frequency shifts. Commun Integr Biol 2, 7–10 (2009).

    Article  Google Scholar 

  67. 67.

    Zanini, D. et al. Proprioceptive Opsin Functions in Drosophila Larval Locomotion. Neuron 98, 67-+, https://doi.org/10.1016/j.neuron.2018.02.028 (2018).

    CAS  Article  PubMed  Google Scholar 

  68. 68.

    Ratnapriya, R. et al. Retinal transcriptome and eQTL analyses identify genes associated with age-related macular degeneration. Nature genetics 51, 606–610, https://doi.org/10.1038/s41588-019-0351-9 (2019).

    CAS  Article  PubMed  PubMed Central  Google Scholar 

  69. 69.

    Schrauwen, I. et al. A comprehensive catalogue of the coding and non-coding transcripts of the human inner ear. Hear. Res. 333, 266–274, https://doi.org/10.1016/j.heares.2015.08.013 (2016).

    CAS  Article  PubMed  Google Scholar 

  70. 70.

    Kaushik, S. & Cuervo, A. M. Proteostasis and aging. Nat. Med. 21, 1406–1415, https://doi.org/10.1038/nm.4001 (2015).

    CAS  Article  PubMed  Google Scholar 

  71. 71.

    Wang, W. W. et al. Impaired unfolded protein response in the degeneration of cochlea cells in a mouse model of age-related hearing loss. Experimental Gerontology 70, 61–70, https://doi.org/10.1016/j.exger.2015.07.003 (2015).

    CAS  Article  PubMed  Google Scholar 

  72. 72.

    Freeman, S. et al. Proteostasis is essential during cochlear development for neuron survival and hair cell polarity. Embo. Rep. 20, 20, https://doi.org/10.15252/embr.201847097 (2019).

    CAS  Article  Google Scholar 

  73. 73.

    Hertzano, R. et al. Cell Type–Specific Transcriptome Analysis Reveals a Major Role for Zeb1 and miR-200b in Mouse Inner Ear Morphogenesis. Plos Genet 7, e1002309, https://doi.org/10.1371/journal.pgen.1002309 (2011).

    CAS  Article  PubMed  PubMed Central  Google Scholar 

  74. 74.

    Nelson, G. Ontogeny, phylogeny, paleontology, and biogenetic law. Systematic Zoology 27, 324–345, https://doi.org/10.2307/2412883 (1978).

    Article  Google Scholar 

  75. 75.

    Richardson, M. K. A Phylotypic Stage for All Animals? Developmental Cell 22, 903–904, https://doi.org/10.1016/j.devcel.2012.05.001 (2012).

    CAS  Article  PubMed  Google Scholar 

  76. 76.

    Kalinka, A. T. et al. Gene expression divergence recapitulates the developmental hourglass model. Nature 468, 811–U102, https://doi.org/10.1038/nature09634 (2010).

    ADS  CAS  Article  PubMed  Google Scholar 

  77. 77.

    Nitta, K. R. et al. Conservation of transcription factor binding specificities across 600 million years of bilateria evolution. Elife 4, https://doi.org/10.7554/eLife.04837 (2015).

  78. 78.

    Sarov, M. et al. A genome-wide resource for the analysis of protein localisation in Drosophila. eLife 5, e12068, https://doi.org/10.7554/eLife.12068 (2016).

    CAS  Article  PubMed  PubMed Central  Google Scholar 

  79. 79.

    Shimada, T., Kato, K., Kamikouchi, A. & Ito, K. Analysis of the distribution of the brain cells of the fruit fly by an automatic cell counting algorithm. Physica A 350, 144–149, https://doi.org/10.1016/j.physa.2004.11.033 (2005).

    ADS  Article  Google Scholar 

  80. 80.

    Ling, D. & Salvaterra, P. M. Robust RT-qPCR Data Normalization: Validation and Selection of Internal Reference Genes during Post-Experimental Data Analysis. Plos One 6, e17762, https://doi.org/10.1371/journal.pone.0017762 (2011).

    ADS  CAS  Article  PubMed  PubMed Central  Google Scholar 

  81. 81.

    Inagaki, H. K., Kamikouchi, A. & Ito, K. Protocol for quantifying sound-sensing ability of Drosophila melanogaster. Nature Protocols 5, 26–30, https://doi.org/10.1038/nprot.2009.206 (2010).

    CAS  Article  PubMed  Google Scholar 

Download references

Acknowledgements

We’d like to thank Ana Carmena de la Cruz (Instituto de Neurociencias, Alicante) and Jürgen Knoblich (IMBA, Vienna) for providing reagents. We are also grateful for fly ageing advice from Linda Partridge and Nathaniel Woodling (UCL Institute of Healthy Ageing, London). We also thank Stefan Németh (SCIMED Illustrations, Vienna) for help with Figure 1a. This work received funding from the Biotechnology and Biological Sciences Research Council (BBSRC), UK (BB/M008533/1 to JTA, AJ and JEG) and BBSRC 16Alert equipment award BB/R000549/1 to JEG, JTA et al.) and from the European Research Council (ERC) under the Horizon 2020 research and innovation programme (Grant agreement Nos 648709 and 862216, both to JTA). CT was supported by a PhD studentship from Action on Hearing Loss, UK (grant S34).

Author information

Affiliations

Authors

Contributions

A.Ke. conducted experiments, analysed data, contributed to the design of experiments and contributed to writing the manuscript. C.T. conducted experiments and analysed data. L.M. conducted experiments and analysed data. A.F. analysed data. A.Ka. conducted experiments and analysed data. F.N. conducted experiments and analysed data. M.G. provided bioinformatical analyses and support J.E.G. contributed to the design of experiments. M.L. contributed to the design of experiments. A.P.J. contributed to the design of experiments and contributed to writing the manuscript. J.T.A. designed and supervised the study, analysed data and wrote the manuscript. All authors reviewed the manuscript.

Corresponding author

Correspondence to Joerg T. Albert.

Ethics declarations

Competing interests

The authors declare no competing interests.

Additional information

Publisher’s note Springer Nature remains neutral with regard to jurisdictional claims in published maps and institutional affiliations.

Supplementary information

Rights and permissions

Open Access This article is licensed under a Creative Commons Attribution 4.0 International License, which permits use, sharing, adaptation, distribution and reproduction in any medium or format, as long as you give appropriate credit to the original author(s) and the source, provide a link to the Creative Commons license, and indicate if changes were made. The images or other third party material in this article are included in the article’s Creative Commons license, unless indicated otherwise in a credit line to the material. If material is not included in the article’s Creative Commons license and your intended use is not permitted by statutory regulation or exceeds the permitted use, you will need to obtain permission directly from the copyright holder. To view a copy of this license, visit http://creativecommons.org/licenses/by/4.0/.

Reprints and Permissions

About this article

Verify currency and authenticity via CrossMark

Cite this article

Keder, A., Tardieu, C., Malong, L. et al. Homeostatic maintenance and age-related functional decline in the Drosophila ear. Sci Rep 10, 7431 (2020). https://doi.org/10.1038/s41598-020-64498-z

Download citation

Comments

By submitting a comment you agree to abide by our Terms and Community Guidelines. If you find something abusive or that does not comply with our terms or guidelines please flag it as inappropriate.

Search

Quick links

Sign up for the Nature Briefing newsletter for a daily update on COVID-19 science.
Get the most important science stories of the day, free in your inbox. Sign up for Nature Briefing