Thermal limits may arise through a mismatch between oxygen supply and demand in a range of animal taxa. Whilst this oxygen limitation hypothesis is supported by data from a range of marine fish and invertebrates, its generality remains contentious. In particular, it is unclear whether oxygen limitation determines thermal extremes in tracheated arthropods, where oxygen limitation may be unlikely due to the efficiency and plasticity of tracheal systems in supplying oxygen directly to metabolically active tissues. Although terrestrial taxa with open tracheal systems may not be prone to oxygen limitation, species may be affected during other life-history stages, particularly if these rely on diffusion into closed tracheal systems. Furthermore, a central role for oxygen limitation in insects is envisaged within a parallel line of research focussing on insect gigantism in the late Palaeozoic.
Here we examine thermal maxima in the aquatic life stages of an insect at normoxia, hypoxia (14 kPa) and hyperoxia (36 kPa). We demonstrate that upper thermal limits do indeed respond to external oxygen supply in the aquatic life stages of the stonefly Dinocras cephalotes, suggesting that the critical thermal limits of such aquatic larvae are set by oxygen limitation. This could result from impeded oxygen delivery, or limited oxygen regulatory capacity, both of which have implications for our understanding of the limits to insect body size and how these are influenced by atmospheric oxygen levels.
These findings extend the generality of the hypothesis of oxygen limitation of thermal tolerance, suggest that oxygen constraints on body size may be stronger in aquatic environments, and that oxygen toxicity may have actively selected for gigantism in the aquatic stages of Carboniferous arthropods.
Citation: Verberk WCEP, Bilton DT (2011) Can Oxygen Set Thermal Limits in an Insect and Drive Gigantism? PLoS ONE 6(7): e22610. https://doi.org/10.1371/journal.pone.0022610
Editor: Alexander W. Shingleton, Michigan State University, United States of America
Received: December 7, 2010; Accepted: July 1, 2011; Published: July 27, 2011
Copyright: © 2011 Verberk, Bilton. This is an open-access article distributed under the terms of the Creative Commons Attribution License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original author and source are credited.
Funding: This study was funded by the Netherlands Organisation for Scientific Research (NWO-RUBICON fellowship no. 825.09.009). The funders had no role in study design, data collection and analysis, decision to publish, or preparation of the manuscript.
Competing interests: The authors have declared that no competing interests exist.
To predict species responses to global warming trends, it is paramount to understand the causal mechanisms underlying thermal limits. The idea of oxygen limitation as a mechanism setting upper thermal limits in animals was first expounded by Winterstein  and has since been greatly expanded by Pörtner and colleagues –. Recent work has extended this principle to lower thermal limits, and sees both upper and lower critical temperatures (CTmax and CTmin) being coupled by the common mechanism of temperature-dependent oxygen limitation. As ectotherms warm the demand for oxygen in their tissues increases faster than the rate at which oxygen can be provided by cardiac and ventilatory processes, leading to a drop in whole-animal aerobic scope and a shift from aerobic to anaerobic metabolism. Similarly on cooling, metabolism slows, leading to insufficient ATP production in ventilatory muscles, reducing oxygen supply to tissues. Deleterious thermal effects are hypothesized to set in first at the whole-animal level, rather than lower hierarchical levels . Thus, temperature-dependent oxygen limitation first lowers whole-animal aerobic scope (and hence performance), followed by the onset of anaerobic metabolism, finally resulting in heat damage to proteins, membranes and cells, and ultimately death , , , .
Although argued to hold for ectotherms in general , most of the evidence for oxygen limitation at thermal extremes to date comes from a variety of marine taxa, including fish, crustaceans, bivalves, and annelids , [ 5 and references therein]. Recent studies of terrestrial isopods and beetles ,  question the generality of this mechanism, suggesting that upper and lower limits are decoupled in terrestrial arthropods, and showing no increase in critical thermal maximum (CTmax) with hyperoxia. Additionally, whilst hypoxia decreased CTmax in isopods, an effect was only seen at extreme hypoxia in beetles, casting doubt on the degree to which oxygen limitation sets upper thermal limits in tracheates. From a functional perspective, both the fact that the tracheal system constitutes a single-step gas exchange system and their high efficiency of oxygen delivery, would indeed seem to preclude oxygen limitation as a major mechanism setting upper thermal limits in terrestrial insects . In addition, terrestrial insects can maintain relatively constant internal oxygen levels, across steep clines in external supply, by adjusting ventilation rates or through compensatory developmental changes in tracheal length, diameter or branching , .
Not all insect species and life-stages may be equally sensitive to temperature-dependent oxygen limitation however and there remains a need for additional studies across the range of morphologies and lifestyles seen in extant insects . In particular, many insects have aquatic larval stages, where the lower oxygen content and diffusion rates in water compared to air dramatically reduce available oxygen , , making oxygen limitation more likely. In addition, larger species or individuals may be more prone to temperature-dependent oxygen limitation because of longer diffusion pathways . Similarly, if body size ultimately constrains an animal's capacity to supply its tissues with oxygen, this would explain why animals attain larger sizes in the cold, where metabolic rates are reduced , . Such size based oxygen limitation is also central to the leading hypothesis regarding insect gigantism in the late Palaeozoic .
Here we provide the first formal test of oxygen limitation in a freshwater tracheate, the stonefly Dinocras cephalotes (Curtis, 1827). Their large, aquatic larvae rely predominantly on tegument respiration, making this an ideal species to study the principle of oxygen limitation. We examine the effects of hypoxia and hyperoxia on CTmax and test whether variation in CTmax amongst individual larvae is related to their oxygen consumption. Given the central role of oxygen in hypotheses on limits to both thermal tolerance and body size , , –, we also discuss how the results of our study may improve our understanding of the role of oxygen in setting body size limits in arthropods. A second reason to discuss insect gigantism, stems from the fact that many insects exhibiting gigantism  apparently had aquatic larvae, although establishing larval lifestyle from fossil data can be difficult , . We do not suggest that insect gigantism is restricted to insects with early aquatic life stages. The now extinct order of Palaeodictyoptera contained several species that displayed marked gigantism and available fossil evidence suggests a terrestrial larval stage , . However, gigantic insects do seem to have been predominantly aquatic; the aquatic larval stage is held to be a common ancestral ground plan  for the giant griffenflies (Protodonata, sometimes also referred to as dragonflies) and giant mayflies (Ephemeroptera) of the late Palaeozoic, as well as the stoneflies (Plecoptera) arising in the Permian. Additionally the gigantic Carboniferous myriapods, the arthopleurids, are usually considered amphibiotic, where the early life stages are aquatic .
To date, attempts to understand insect gigantism in the late Palaeozoic have mainly been approached from the perspective of (fossilized) terrestrial adults. Yet, if oxygen limitation at thermal extremes operates differently for aquatic larvae and terrestrial adults, approaching the problem of historical gigantism from a larval perspective instead may similarly shed new light on the possible role of oxygen in setting insect body size limits. A larval view seems furthermore promising as insects with aquatic larval stages can circumvent the problem of structural support during their growing phase , while their flying adults overcome leg space limitations governing tracheal space limitations in walking insects .
Here we demonstrate that upper thermal limits in the aquatic life stages of an insect do indeed respond to external oxygen supply and that these are related to the oxygen consumption of individual larvae. These findings extend the generality of the hypothesis of oxygen limitation of thermal tolerance, suggest that oxygen constraints on body size may be stronger in aquatic environments, and that oxygen toxicity may have actively selected for gigantism in the aquatic stages of Carboniferous arthropods.
Critical thermal maximum (CTmax) differed significantly across oxygen treatments (Table 1) being raised by 1·53°C in hyperoxia and lowered by 2·92°C in hypoxia (Fig. 1A). Individual larvae differed in thermal sensitivity for oxygen consumption rates (expressed by Q10 values), which significantly affected their CTmax (Table 1). Thermal maxima were approximately 1°C lower for individuals with a high thermal sensitivity (Q10 value of 3) compared to individuals with a low thermal sensitivity (Q10 value of 1) (Fig. 1B). While we did not find a direct relationship between body mass and CTmax (Table 1; Fig. 1C), larger instars had higher Q10 values in comparison to smaller instars (t-test, t1,41 = 2·19, P = 0·038). This suggests that potential effects of body mass are mediated primarily through increased thermal sensitivity, something which seems most apparent at hypoxia (Fig. 1C).
Differences in CTmax were consistent with the mechanism of oxygen limitation: hypoxia lowered CTmax, while hyperoxia increased CTmax (a) and thermal maxima were lower for individuals which strongly increased their oxygen consumption rates at higher temperatures (high Q10 values). Each bar represents the average (± s.e.) of 15 nymphs. Letters indicate significant differences (P<0.05; Tukey HSD post hoc test following an anova including only oxygen treatment: F2,41 = 44·06, P<0·001).
Here we find strong evidence for the idea that a mismatch between external oxygen supply and internal oxygen demand can set thermal limits in aquatic insects : hypoxia lowered thermal maxima, whilst hyperoxia increased them (Fig. 1A). At the same time, individuals that strongly increased oxygen consumption at elevated temperatures had lower thermal maxima (Fig. 1B). These results contrast with previous investigations on terrestrial adult insects, and provide a proof of principle that oxygen limitation can set upper thermal limits in aquatic insect larvae. Drawing on differences in ontogeny (closed trachea) and ecology (aquatic habitat), two explanations could be made for the apparent mismatch between oxygen supply and demand in the stonefly nymphs, causing the onset of oxygen limitation at thermal extremes.
First, oxygen delivery may be impeded in stonefly nymphs because of their closed tracheae and because of the lower oxygen content and diffusion rates in water compared to air. At higher temperatures, more oxygen is available to an aquatic organism because of the higher diffusivity of oxygen, yet scope for aerobic metabolism is nevertheless reduced as increases in organismal oxygen demand exceed increases in oxygen supply . Although a closed tracheal system still represents a one-stage oxygen delivery system, oxygen delivery is more likely to become rate limiting at higher temperatures because of the additional step of oxygen diffusion across the epithelium. The absence of air sacs in larvae may further limit oxygen delivery rates by increasing the relative importance of diffusive rather than convective movement of oxygen in the trachea , although the compression and expansion of the trachea themselves  may in some cases generate substantial convective movement . An increased difficulty of oxygen delivery in an aquatic environment fits with the fact that CTmax at normoxia is generally reported to be higher for terrestrial than aquatic arthropod life stages , , –. As CTmax is reached at lower temperatures in aquatic taxa, this is less likely to be a result of thermal damage at the cellular level such as the disruption of membrane structure and problems associated with protein folding , , which would make oxygen limitation more decisive in setting thermal limits in aquatic life stages, rather than one of several factors as suggested for terrestrial insects , . One assumption here is that aquatic taxa have not considerably altered their membrane fluidity and protein activity in response to the more stable, often lower thermal regime in aquatic habitats (see below). If oxygen is more important at less extreme thermal maxima relative to other factors (membrane fluidity and protein stability), it would explain why CTmax increased with hyperoxia in the stonefly nymphs studied here (Fig. 1A) and in aquatic mayfly nymphs studied by Whitney , but not in the terrestrial tracheates with open tracheal systems studied so far , .
Second, changes in external oxygen levels may have stronger impacts on internal oxygen levels in aquatic invertebrates, and hence thermal tolerance, if their oxygen regulatory capacity is more limited than that of terrestrial invertebrates. Insects are forced to regulate internal oxygen levels within a fairly narrow range, balancing the risk of asphyxiation with that of oxygen toxicity , , . Whereas terrestrial insects can simply open or close spiracles to regulate oxygen uptake, such regulation is unavailable to aquatic stages with closed tracheal systems such as Dinocras. Equally, fluctuations in ectotherm oxygen consumption are reduced in aquatic habitats owing to their thermally buffered nature. In short, the ability to regulate internal oxygen levels is inherently limited in taxa with closed tracheal systems, while the need to do so is lower in aquatic habitats. With poor regulation of oxygen intake in Dinocras, it is perhaps not too surprising to find a relationship between CTmax of individual stonefly nymphs and their thermal sensitivity in oxygen consumption (Fig. 1B). As these measurements of oxygen consumption were performed at ecologically realistic temperatures, aerobic scope for feeding, growth and reproduction may be likewise affected by the interplay between external oxygen supply and organismal oxygen demand, although the thermal limits associated with these performance measures will be lower than those for the short-term survival reported here , , .
In each of the above explanations the conditions that make oxygen limitation more likely arise from both the aquatic nature (lower oxygen availability and higher thermal buffering) and the closed tracheal system (limiting oxygen delivery and regulatory capacity). Consequently, oxygen limitation may be especially likely for insects that have life stages with closed tracheal systems and live in an aquatic or essentially aquatic environment (e.g. endoparasites, endophytic species, some rotten wood borers, rotten fruit specialists, etc.). Thus, many insects may be affected by oxygen limitation at some stage during their life cycle; indeed different life stages vary in their susceptibility to hypoxia , ,  and thermal tolerance .
Similarly, both of the above explanations for the onset of oxygen limitation at thermal extremes could underlie insect gigantism. While they do not preclude additional evolutionary routes toward gigantism (which seems most probable for entirely terrestrial taxa like the Palaeodictyoptera), they could explain why gigantism was apparently frequent amongst arthropods with juvenile aquatic life stages. Importantly, each explanation makes very different predictions. The first, of impeded oxygen delivery, follows the existing explanation that increased atmospheric levels of oxygen in the late Palaeozoic permitted the evolution of larger body sizes. The basic difference is that oxygen limitation first sets in at the larval stage, either owing to the lower availability of oxygen in water compared to air ,  or the additional barrier of diffusion across the epithelium.
Oxygen limitation in larvae fits with the observation that oxygen delivery does not seem to become much more challenging for larger bodied adults of terrestrial insects , . Although larger animals are predicted to be more prone to oxygen limitation, such size dependency may only be evident under certain conditions , , given that larger individuals may have modified respiratory structures, and change their respiratory behaviour to compensate for reductions in oxygen supply capacity associated with larger size , . Costs associated with such compensatory changes may include tracheal hypertrophy , , or increased thermal sensitivity (see results). These costs may be reflected in the long term, underlying observed variation in body size across environmental gradients of temperature or oxygen availability , . Here we found support for size related performance in the hypoxic treatment only (Fig. 1C). A possible explanation for this is that the tracheal network of the larger individuals, which developed under normoxia in the field, was of insufficient capacity when larvae approached their thermal limits under hypoxia. At higher levels of oxygen, other limits may have set in that were less dependent on size, involving the failure of oxygen delivery systems operating at the cellular level .
A fundamental problem with a passive oxygen ceiling constraining maximum body size is that it is inferred from extant taxa having physiologies optimized to normoxic conditions and therefore may not reflect the evolutionary limit of tracheal breathing . The second explanation of limited oxygen regulatory capacity recasts oxygen as an active driver of gigantism by focussing on the risks of having too much oxygen, rather than too little. In aquatic larvae with closed tracheal systems and limited ability to regulate internal oxygen levels, internal oxygen levels would be expected to closely track environmental oxygen levels. Whilst species are likely to have experienced and evolved responses to cope with periods of hypoxia , the same may not apply for hyperoxia, putting aquatic larvae at greater risk of oxygen poisoning than terrestrial adults . If large body sizes are more sensitive to hypoxia and asphyxiation, they may equally confer protection from oxygen toxicity , constituting an antioxidant response .
In support of oxygen as an active driver of increasing body size, Loudon  found that beetle larvae increased in body mass when they were transferred from hypoxia to normoxia during their development. The logic is that larvae which started their development in hypoxia increased their tracheal size, but could not decrease them again upon returning to normoxia, as the new trachea are built around the old trachea of the previous larval instar. Although increasing body mass entails costs, body mass results from the net effect of many different factors . During development, internal hypoxia acts as a signal and may stimulate tissue differentiation instead of growth, thus affecting the size reached. Similarly hyperoxia may trigger an increase in body size as a readily available way to effectively escape oxygen toxicity, possibly enabled through lower costs in ventilation or tracheal investments , , . Hence hyperoxia may actively drive evolutionary increases in body mass, even in small insects . Direct evidence for oxygen toxicity in a range of freshwater invertebrate species is provided by Fox & Taylor  who found that smaller juvenile stages are more sensitive to hyperoxic conditions than their larger aquatic adults.
An active selection for larger body sizes under hyperoxia would fit with the reappearance of giant mayflies in the putative high oxygen atmosphere at the end-Cretaceous  and the persistence of giant insects during putative lower levels of atmospheric oxygen. Examples of the latter include large griffenflies (Protodonata) in the late Permian  and abnormally large dragonflies (Odonata) during the Triassic/Jurassic . Similarly, oxygen as an active driver of gigantism would predict a shift in size spectra such that average size increases, rather than a unilateral broadening of size spectra where only the body size of the largest species increases, as predicted by a passive oxygen ceiling. While establishing changes in modal sizes from the fossil record is fraught with difficulties, size spectra in extant amphipod assemblages would support oxygen as an active driver, where not only maximum body size within an assemblage, but also average and even minimum body size is greater at higher ratios of oxygen supply to demand , .
Thus, a larval view of Paleozoic hyperoxia-enabled gigantism in insects may be very informative. We suggest the aquatic larval stage as a route to gigantism, explaining the predominance of aquatic life stages amongst extinct gigantic insects. In aquatic juvenile stages, impeded oxygen delivery may have resulted in stronger constraints on body size, whilst larger body sizes may have been actively selected for to avert oxygen toxicity. The widespread gigantism in marine species further supports this hypothesis, with examples of gigantism ,  found predominantly at times when oxygen levels were perhaps not higher than current ones, but rising , effectively putting the animals at risk of oxygen poisoning. Each of the two explanations for a larger role of oxygen in aquatic stages yields testable predictions concerning the relative rates of evolution of larger and smaller body sizes, and the shifting or broadening size spectra.
Materials and Methods
Animals were collected from the River Dart, Devon, UK and maintained in the lab at 10±1°C in a 12 L∶12 D regime. They were kept in a flow-through aquarium (10 L·min−1), fed with artificial pond water , buffered and diluted to reflect the pH and conductivity of the field site (pH 6.4–6.6, 70–150 µS·cm−1) and fed chironomid larvae. Oxygen consumption was measured for each larva at 10°C and 15°C using closed glass respiration chambers of 67.5–68.5 ml. The chambers were immersed in a temperature controlled bath (±0.1°C) and stirred using underwater magnetic stirrers to ensure mixing of water. Respiration chambers were fitted with a fine nylon mesh forming a false bottom to prevent contact between the larvae and the magnetic stirrer bar. Individuals were allowed to acclimate for 10 min before the chambers were closed and left for 60 min. Oxygen content was measured before and after using an O2 electrode (1302 Oxygen Electrode, Strathkelvin Instruments) that was connected to a calibrated meter (Oxygen Meter 929, Strathkelvin Instruments). On average, larvae depleted oxygen levels only by 5% (with a maximum of 18%) and oxygen consumption was expressed as µg O2 (mg wet mass)−1 h−1. Oxygen consumption of larvae at 10°C was significantly correlated with their consumption at 15°C (Partial correlation, corrected for differences in body mass: r = 0.511, P<0.001), justifying the calculation of Q10 values for individuals. One individual was removed from further analysis as abnormally low oxygen consumption measured at 10°C resulted in an unrealistic Q10 value of 99.The Q10 values calculated for each specimen were correlated with the CTmax values of the exact same individuals.
To assess CTmax at normoxia, animals were placed in small flow-through chambers (70×70×30 mm; flowrate 0.016 L·s−1) fed with water from a 25 L header tank passing through a tubular counter current heat exchanger. Water in the header tank was of the same composition as that used to maintain animals, and was bubbled with a mixture of 20% oxygen and 80% nitrogen, obtained using a gas-mixing pump (Wösthoff, Bochum, Germany), and covered with 18 mm thick expanded polystyrene sheeting to prevent equilibration with the atmosphere. Before the start of the experiment, animals were left to acclimate for 1 h at the starting temperature of 10°C, after which temperature in the experimental chambers was increased at 0.25°C min−1, using a Grant R5 water bath with a GP200 pump unit (Grant Instrument (Cambridge) Ltd, UK), connected to the heat exchanger. Temperatures were logged using a HH806AU digital thermometer (Omega Engineering Inc., USA). CTmax was recorded as the point at which animals no longer showed any body movement or muscular spasms. Animals which were at this point transferred to fully oxygenated water of 10°C recovered with no apparent lasting damage. Below critical maxima, larvae initiated in repeated swimming behaviour (around 29°C; interpreted as attempts to escape experimental conditions) and fell upon their backs (around 30°C) and an onset of spasms was observed (around 31°C). We used a dynamic method (acute exposure to changing temperatures) in contrast to most work performed on marine taxa, which used static methods (chronic exposure to constant temperatures , ). As faster rates of warming can result in higher critical thermal maxima , , we employed the same rate of warming as employed in previous studies on terrestrial insects to minimize confounding effects arising from methodological differences in a direct comparison of our results with theirs. To assess CTmax at hypoxia (5% O2, 95% N2) and hyperoxia (60% O2, 40% N2), the gas mixture was adjusted 10 min after placing the animals in the small flow-through chambers. In this way animals were gradually exposed to hypoxic and hyperoxic conditions during acclimation. In several test runs, oxygen levels were measured after adjusting the gas mixture to determine when and at which value oxygen levels stabilized. From these measurements the relative contributions of the gas mixture and normal air to the (hypoxic or hyperoxic) test water could be determined. The oxygen levels stabilised after 1 hour at 36 kPa (34–38) and 14 kPa (13.3–14.8) for the hyperoxia and hypoxia treatment, respectively.
We thank Andrew Atfield, Roger Haslam, Rick Preston, Peter Russell, Richard Ticehurst and Saar Verberk for logistic support. Two anonymous referees made critical, much appreciated comments that improved the manuscript.
Conceived and designed the experiments: WV DB. Performed the experiments: WV. Analyzed the data: WV. Wrote the paper: WV DB.
- 1. Winterstein H (1905) Wärmelähmung und Narkose. Z Allg Physiol 5: 323–350.
- 2. Frederich M, Pörtner HO (2000) Oxygen limitation of thermal tolerance defined by cardiac and ventilatory performance in spider crab, Maja squinado. Am J Physiol – Regul Integr Comp Physiol 279: R1531–R1538.
- 3. Pörtner HO (2002) Climate variations and the physiological basis of temperature dependent biogeography: systemic to molecular hierarchy of thermal tolerance in animals. Comp Biochem Physiol A 132: 739–761. (doi:10.1016/S1095-6433(02)00045-4).
- 4. Pörtner HO (2006) Climate-dependent evolution of Antarctic ectotherms: An integrative analysis. Deep-Sea Res II 53: 1071–1104. (doi:10.1016/j.dsr2.2006.02.015).
- 5. Pörtner HO (2010) Oxygen- and capacity-limitation of thermal tolerance: a matrix for integrating climate-related stressor effects in marine ecosystems. J Exp Biol 213: 881–893. (doi:10.1242/jeb.037523).
- 6. Pörtner HO (2001) Climate change and temperature-dependent biogeography: oxygen limitation of thermal tolerance in animals. Naturwissenschaften 88: 137–146. (doi:10.1007/s001140100216).
- 7. Stevens MM, Jackson S, Bester SA, Terblanche JS, Chown SL (2010) Oxygen limitation and thermal tolerance in two terrestrial arthropod species. J Exp Biol 213: 2209–2218. (doi:10.1242/jeb.040170).
- 8. Klok CJ, Sinclair BJ, Chown SL (2004) Upper thermal tolerance and oxygen limitation in terrestrial arthropods. J Exp Biol 207: 2361–2370. (doi:10.1242/jeb.01023).
- 9. Loudon C (1989) Tracheal hypertrophy in mealworms: Design and plasticity in oxygen supply systems. J Exp Biol 147: 217–235.
- 10. Harrison JF, Frazier MR, Henry JR, Kaiser A, Klok CJ, et al. (2006) Responses of terrestrial insects to hypoxia or hyperoxia. Resp Physiol Neurobiol 154: 4–17. (doi:10.1016/j.resp.2006.02.008).
- 11. Lighton JRB (2007) Hot hypoxic flies: Whole-organism interactions between hypoxic and thermal stressors in Drosophila melanogaster. J Therm Biol 32: 134–143. (doi:10.1016/j.jtherbio.2007.01.009).
- 12. Jones JD (1972) Comparative Physiology of Respiration. Special Topics in Biology Series. London: Edward Arnold Ltd.
- 13. Verberk WCEP, Bilton DT, Calosi P, Spicer JI (2011) Oxygen supply in aquatic ectotherms: Partial pressure and solubility together explain biodiversity and size patterns. Ecology 92: 1565–1572. (doi:10.1890/10-2369.1).
- 14. Atkinson D, Morley SA, Hughes RN (2006) From cells to colonies: at what levels of body organization does the ‘temperature-size rule’ apply? Evol Dev 8: 202–214. (doi: 10.1111/j.1525-142X.2006.00090.x).
- 15. Harrison JF, Kaiser A, VandenBrooks JM (2010) Atmospheric oxygen level and the evolution of insect body size. Proc R Soc Lond B 277: 1937–1946. (doi:10.1098/rspb.2010.0001).
- 16. Chapelle G, Peck L (1999) Polar gigantism dictated by oxygen availability. Nature 399: 114–115. (doi:10.1038/20099).
- 17. Woods HA, Moran AL, Arango CP, Mullen L, Shields C (2009) Oxygen hypothesis of polar gigantism not supported by performance of Antarctic pycnogonids in hypoxia. Proc R Soc Lond B 276: 1069–1075. (doi:doi:10.1098/rspb.2008.1489).
- 18. Graham JB, Dudley R, Aguilar NM, Gans C (1995) Implications of the late Palaeozoic oxygen pulse for physiology and evolution. Nature 375: 117–120. (doi: 10.1038/375117a0).
- 19. Wootton RJ (1988) The historical ecology of aquatic insects: an overview. Palaeogeogr Palaeoclim Palaeoecol 62: 477–492. (doi:10.1016/0031-0182(88)90068-5).
- 20. Kukalová-Peck J (1983) Origin of the insect wing and wing articulation from the arthropodan leg. Can J Zool 61: 1618–1669. (doi:10.1139/z83-217).
- 21. Wootton RJ (1972) Nymphs of Palaeodictyoptera (Insecta) from the Westphalian of England. Paleontology 15: 662–675.
- 22. Shear WA, Kukalová-Peck J (1990) The ecology of Paleozoic terrestrial arthropods: the fossil evidence. Can J Zool 68: 1807–1834. (doi:10.1139/z90-262).
- 23. Kaiser A, Klok CJ, Socha JJ, Lee W-K, Quinlan MC, et al. (2007) Increase in tracheal investment with beetle size supports hypothesis of oxygen limitation on insect gigantism. Proc Natl Acad Sci USA 104: 13198–13203. (doi:10.1073/pnas.0611544104).
- 24. Westneat MW, Betz O, Blob RW, Fezzaa K, Cooper WJ, et al. (2003) Tracheal respiration in insects visualized with synchrotron X-ray imaging. Science 299: 558–560. (doi:10.1126/science.1078008).
- 25. Socha JJ, Lee W-K, Harrison JF, Waters JS, Fezzaa K, et al. (2008) Correlated patterns of tracheal compression and convective gas exchange in a carabid beetle. J Exp Biol 211: 3409–3420. (doi:10.1242/jeb.019877).
- 26. Whitney RJ (1939) The Thermal Resistance of Mayfly Nymphs from Ponds and Streams. J Exp Biol 16: 374–385.
- 27. Chown SL (2001) Physiological variation in insects: hierarchical levels and implications. J Ins Physiol 47: 649–660. (doi:10.1016/S0022-1910(00)00163-3).
- 28. Calosi P, Bilton DT, Spicer JI, Atfield A (2008) Thermal tolerance and geographical range size in the Agabus brunneus group of European diving beetles (Coleoptera: Dytiscidae). J Biogeogr 35: 295–305. (doi:10.1111/j.1365-2699.2007.01787.x).
- 29. Wijnhoven S, van Riel MC, van der Velde G (2003) Exotic and indigenous freshwater gammarid species: physiological tolerance to water temperature in relation to ionic content of the water. Aquat Ecol 37: 151–158. (doi:10.1023/A:1023982200529).
- 30. Feder ME, Hofmann GE (1999) Heat-shock proteins, molecular chaperones, and the stress response:Evolutionary and Ecological Physiology. Annu Rev Physiol 61: 243–82. (doi:10.1146/annurev.physiol.61.1.243).
- 31. Somero GN (2004) Adaptation of enzymes to temperature: searching for basic “strategies”. Comp Biochem Physiol B 139: 321–333. (doi:10.1016/j.cbpc.2004.05.003).
- 32. Fox HM, Taylor AER (1955) The tolerance of oxygen by aquatic invertebrates. Proc R Soc Lond B 143: 214–225. (doi:10.1098/rspb.1955.0006).
- 33. Hetz SK, Bradley TJ (2005) Insects breathe discontinuously to avoid oxygen toxicity. Nature 433: 516–519. (doi:10.1038/nature03106).
- 34. Woods HA, Hill RI (2004) Temperature-dependent oxygen limitation in insect eggs. J Exp Biol 207: 2267–2276. (doi:10.1242/jeb.00991).
- 35. Klok CJ, Kaiser A, Lighton JRB, Harrison JF (2010) Critical oxygen partial pressures and maximal tracheal conductances for Drosophila melanogaster reared for multiple generations in hypoxia or hyperoxia. J Ins Physiol 56: 461–469. (doi:10.1016/j.jinsphys.2009.08.004).
- 36. Marais E, Terblanche JS, Chown SL (2009) Life stage-related differences in hardening and acclimation of thermal tolerance traits in the kelp fly, Paractora dreuxi (Diptera, Helcomyzidae). J Ins Physiol 55: 336–343. (doi:10.1016/j.jinsphys.2008.11.016).
- 37. Butterfield NJ (2009) Oxygen, animals and oceanic ventilation: an alternative view. Geobiol 7: 1–7. (doi:10.1111/j.1472-4669.2009.00188.x).
- 38. Hoback WW, Stanley DW (2001) Insects in hypoxia. J Ins Physiol 47: 533–542. (doi: 10.1016/S0022-1910(00)00153-0).
- 39. Van Voorhies WA (2009) Metabolic function in Drosophila melanogaster in response to hypoxia and pure oxygen. J Exp Biol 211: 3409–3420. (doi:10.1242/jeb.031179).
- 40. Klok CJ, Hubb AJ, Harrison JF (2009) Single and multigenerational responses of body mass to atmospheric oxygen concentrations in Drosophila melanogaster: evidence for roles of plasticity and evolution. J Evol Biol 22: 2496–2504. (doi:10.1111/j.1420-9101.2009.01866.x).
- 41. Lane N (2002) Oxygen: The Molecule that made the World. Oxford: Oxford University Press.
- 42. Owerkowicz T, Elsey RM, Hicks JW (2009) Atmospheric oxygen level affects growth trajectory, cardiopulmonary allometry and metabolic rate in the American alligator (Alligator mississippiensis). J Exp Biol 212: 1237–1247. (doi:10.1242/jeb.023945).
- 43. Grimaldi D, Engel MS (2005) Evolution of the Insects. New York: Cambridge University Press.
- 44. Nel AN, Fleck G, Garrouste R, Gand G (2008) The Odonatoptera of the Late Permian Lodève Basin (Insecta). J Iberian Geol 34: 115–122.
- 45. Okajima R (2008) The controlling factors limiting maximum body size of insects. Lethaia 41: 423–430. (doi:10.1111/j.1502-3931.2008.00094.x).
- 46. Chapelle G, Peck LS (2004) Amphipod crustacean size spectra: new insights in the relationship between size and oxygen. Oikos 106: 167–175. (doi:10.1111/j.0030-1299.2004.12934.x).
- 47. Rudkin DM, Young GA, Elias RJ, Dobrzanski EP (2003) The world's biggest trilobite – Isotelus rex new species from the Upper Ordovician of northern Manitoba, Canada. J Paleont 77: 99–112.
- 48. Braddy SJ, Poschmann M, Tetlie OE (2008) Giant claw reveals the largest ever arthropod. Biol Lett 4: 106–109. (doi: 10.1098/rsbl.2007.0491).
- 49. Berner RA, VandenBrooks JM, Ward PD (2007) Oxygen and Evolution. Science 316: 557–558.
- 50. ASTM (1980) Standard practice for conducting acute toxicity tests with fishes, macroinvertebrates and amphibians. American standard for testing and materials, Philadelphia, Pennsylvania, USA 279–280.
- 51. Terblanche JS, Deere JA, Clusella-Trullas S, Janion C, Chown SL (2007) Critical thermal limits depend on methodological context. Proc R Soc Lond B 274: 2935–2942. (doi:10.1098/rspb.2007.0985).
- 52. Peck LS, Clark MS, Morley SA, Massey A, Rossetti H (2009) Animal temperature limits and ecological relevance: effects of size, activity and rates of change. Funct Ecol 23: 248–256. (doi: 10.1111/j.1365-2435.2008.01537.x).